Eastman Chemical Company has a position in its corporate research and development labs for a microscopist. Extensive experience with both optical and electron microscopy is required and experience in AFM, computer programming, and/or particle size analysis would be a strong plus. Knowledge of polymer morphology and/or the morphology of coatings and inks is also highly desirable. A PhD is preferred. The laboratory is well equipped with several optical microscopes, an SEM, a TEM, an AFM, and a particle size analyzer. The successful candidate will be working with this equipment and other scientists and engineers at Eastman to develop new/improved polymers and chemicals and to help solve manufacturing problems. Candidates must be highly motivated, have good communication skills and be able to work with teams.
Eastman Chemical Company, a Fortune 500 company, is a major manufacturer of plastics, fibers, and specialty organic chemicals. This position is at the Kingsport, TN site. Kingsport is located in northeast Tennessee in the foothills of the Smoky Mountains. It is Eastman's policy to provide equal opportunity for all qualified persons; to prohibit unlawful discrimination in employment practices, compensation practices, personnel procedures, and the administration of benefit plans and other programs; and to promote a full realization of equal employment opportunity through continuing affirmative action throughout company establishments. Reference Requisition No. 723 in your cover letter. Send CV/Resume to lmotz-at-eastman.com {mailto:lmotz-at-eastman.com} or to Eastman Chemical Company, PO Box 1975, B-215 - Staffing, Attn: Laurie Motz, Kingsport, TN 37662.
} Louis T. Germinario (Lou) } Physical Chemistry Research Laboratory } Eastman Chemical Company } Lincoln Street, B-150B } P.O. Box 1972 } Kingsport, TN 37662-5150 } (423) 229-4047 } (423) 229-4558 (Fax) } mailto:germ-at-eastman.com } }
Peter, I don't believe the original message is proposing the method you used. Many companies (including my own) provide EDX/imaging upgrades that replace the EDX system except for the detector and detector preamp. On most detectors, these upgrades are very easy to install.
Regarding the imaging, older SEMs vary even within the same model number. The Hitachi S570 is sometimes equipped to readily accept an active-scan system. We've seen others that require the installation of a Hitachi digital beam control box. With an active-scan system, older SEMs can acquire high-resolution digital images of amazing quality. Prices vary greatly and typically depend on the software requirements (i.e. acquisition and analysis, versus just acquisition).
Beth Gregory 4pi Analysis, Inc.
} Todd; } } I have done as you mentioned on a Hitachi S570. That is, used the EDX } system's imaging and beam control as a capture vehicle. The only issue at } the time was the resolution of the captured image relative to acquisition } time since the processing capability was based on an old microprocessor and } motherboard in the EDX hardware. In the older SEMs such as the Hitachi } S570, there is no readily available port to grab the horizontal and vertical } scan information and hence the video board had to be physically spliced into } and the electronic levels made compatible with the EDX electronics. It was } a messy affair but ultimately did work. The system worked on a Win95 } platform. } } The cost to do this on your particular microscope will likely be a function } of who will be doing it, EDX vendor or graduate student. If you have an } electrical engineering dept., you may want to tap into that resource for a } good EE type person that understands analog/digital interfaces. } } Hope this is of some aid. } } Peter Tomic } } -----Original Message----- } } From: Todd Kostman [mailto:kostman-at-vaxa.cis.uwosh.edu] } Sent: Wednesday, August 28, 2002 12:58 PM } To: Microscopy-at-sparc5.microscopy.com } Subject: conversion of SN-2460 to digital } } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
You can also try growing them on a 100 mm plate. I have done this after the osmification and using a rubber cell scraper, gently removed enough cells to get a visible pellet. Also check the plate under phase microscopy to ensure cell numbers.
Mike D.
"Sherwood, Margaret" wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } Have you thought about growing them on a coverslip and then processsing the } cells intact--the final stage would involve inverting a beem capsule with } epon on top of it, polymerizing it, and then using liquid nitrogen to pop } the capsul off. Cells adhere nicely to the epon and then you can section. } } Peggy Sherwood } Lab Associate, Photopathology } Wellman Laboratories of Photomedicine (W224) } Massachusetts General Hospital } 55 Fruit Street } Boston, MA 02114 } 617-724-4839 (voice mail) } 617-726-6983 (lab) } 617-726-3192 (fax) } msherwood-at-partners.org } } } -----Original Message----- } } From: Leslie Cummins [SMTP:gunther-at-aecom.yu.edu] } } Sent: Monday, August 26, 2002 3:01 PM } } To: Microscopy-at-sparc5.microscopy.com } } Subject: TEM - macrophage collection } } } } ------------------------------------------------------------------------ } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } } -----------------------------------------------------------------------. } } } } } } Hello Listers } } } } I am having a problem attempting to scrape and collect primary macrophage } } grown on a 60mm plastic petri dish. } } } } The cells are fixed in 4% paraformaldehyde, blocked with 0.05M glycine, } } buffer rinsed, then water rinsed. I am using a disposable cell scraper } } from Fisher and scraping them in a very small amount of water, almost } } dry. When I collect the water with a pipet and transfer to an eppendof } } tube to spin the pellet down, there seem to be no cells. I have tried } } spinning them very hard, or very long but to no avail. I use this } } protocol } } on other cell types and get wonderful pellets, with plenty of sample to } } work with. } } } } It seems to be cell type specific and I was wondering if anyone had any } } ideas to help me get a usable, visible pellet. I am trying to do } } ultrathin } } cryosections, so I am slightly limited in my options. } } } } Thanks in advance. } } Leslie } } } } } } } } Leslie Gunther Cummins } } Analytical Imaging Facility } } Albert Einstein College of Medicine } } 1300 Morris Park Ave. } } Bronx, NY 10461 } } 718-430-3547 } } } } http://www.aecom.yu.edu/aif/ } }
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Beth, all,
Considering the fact that the SEM already has an EDS system attached, I would guess, that it is already equipped with the digital beam control interface. That would probably allow to hook up any of the digital acquisition systems, yours, ours, etc.
A possibly more cost efficient way might be to talk to Noran and see if they have a migration possibility from this Unix system to a PC based system. Noran is using our software on some of their systems, so that might be a possibility to get image acquisition on a PC and some processing capabilities at the same time. However, depending on the age of the system, that might not be possible, or only with additional hardware changes.
If only image acquisition is required, our ADDA II can be operated in parallel to an existing EDS system (I am sure your system can do that also), with options do to dot mapping.
mike
Michael Bode, Ph.D. Soft Imaging System Corp. 12596 West Bayaud Avenue Suite 300 Lakewood, CO 80228 =================================== phone: (888) FIND SIS (303) 234-9270 fax: (303) 234-9271 email: mailto:info-at-soft-imaging.com web: http://www.soft-imaging.com ===================================
******* Disclaimer ******** As the manufacturer of digital image acquisition systems we DO have an interest (financial and otherwise) in the products mentioned above. Please make sure to get all information before making a decision. **************************
-----Original Message----- } From: Beth Gregory [mailto:gregory-at-4pi.com] Sent: Thursday, August 29, 2002 8:41 AM To: Microscopy-at-sparc5.microscopy.com
Peter, I don't believe the original message is proposing the method you used. Many companies (including my own) provide EDX/imaging upgrades that replace the EDX system except for the detector and detector preamp. On most detectors, these upgrades are very easy to install.
Regarding the imaging, older SEMs vary even within the same model number. The Hitachi S570 is sometimes equipped to readily accept an active-scan system. We've seen others that require the installation of a Hitachi digital beam control box. With an active-scan system, older SEMs can acquire high-resolution digital images of amazing quality. Prices vary greatly and typically depend on the software requirements (i.e. acquisition and analysis, versus just acquisition).
Beth Gregory 4pi Analysis, Inc.
} Todd; } } I have done as you mentioned on a Hitachi S570. That is, used the EDX } system's imaging and beam control as a capture vehicle. The only issue at } the time was the resolution of the captured image relative to acquisition } time since the processing capability was based on an old microprocessor and } motherboard in the EDX hardware. In the older SEMs such as the Hitachi } S570, there is no readily available port to grab the horizontal and vertical } scan information and hence the video board had to be physically spliced into } and the electronic levels made compatible with the EDX electronics. It was } a messy affair but ultimately did work. The system worked on a Win95 } platform. } } The cost to do this on your particular microscope will likely be a function } of who will be doing it, EDX vendor or graduate student. If you have an } electrical engineering dept., you may want to tap into that resource for a } good EE type person that understands analog/digital interfaces. } } Hope this is of some aid. } } Peter Tomic } } -----Original Message----- } } From: Todd Kostman [mailto:kostman-at-vaxa.cis.uwosh.edu] } Sent: Wednesday, August 28, 2002 12:58 PM } To: Microscopy-at-sparc5.microscopy.com } Subject: conversion of SN-2460 to digital } } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (cbc-at-post.queensu.ca) from http://www.msa.microscopy.com/Ask-A-Microscopist.html on Thursday, August 29, 2002 at 11:02:32 ---------------------------------------------------------------------------
Email: cbc-at-post.queensu.ca Name: Charlie Cooney
Organization: Queens University
Education: Graduate College
Location: Kingston, Ontario Canada
Question: I have been doing some housekeeping and came across a bottle of Dr. Vogel's Sparbeize. My recollection is that this was an additive to an electropolishing solution for metals but I cannot remember what the chemical compostion of this stuff is or what solution it was use in. Does anyone know how to use this stuff and what the compositon is?
I need to find a good adhesive to use as for plastic serial sections. One recommendation was a product called Pattex diluted with xylene. I am unable to locate this product.
Any other suggestions for accomplishing good serial sections? I'm using a diamond histo knife with big boat.
Thanks, Tim Quinn University of Kansas Program Assistant/Microscopists Ornithology Dept. Natural History Museum and Biodiversity Research Center Dyche Hall Room 414 Lawrence, KS 6604-2454 785-864-4556/785-331-4107 tquinn-at-ku.edu
Sparbeize is indeed an additive to other etching solutions. It was produced by a German company. (Max Hoeck o.H.G. in Duesseldorf). It was used for etching mainly stainless steel samples with a high Cr content. eg. 10 ccs HNO3 0.30 Vogels Sparbeize 100 ccs HCL 100 ccs dist H2O Etching either at room temp or 50 degrees C. As I can remember, the actual ingredients of Sparbeize were kept secret.
Cheers
Hans Brinkies Professional Officer, Electron Microscopy and Metallography Swinburne, University of Technology School of Engineering and Science Industrial Microscopy Laboratory P.O.Box 218 - Hawthorn - Vic -3122 - Australia Phone: +61 3 9214 8657 Fax: +61 3 9214 8264 Email: Hbrinkies-at-swin.edu.au
Thanks to everybody who replied to my question. I started off answering each reply individually, but there are just so many that I hope everybody will accept this blanket gratitude. It seems to be a common problem among EM people and other microscopists, so perhaps it could count as an occupational injury. If it is, please everybody, take care to prevent it, as far as you can.
pattex is a subdivision of Henkel / Germany. - I do not know if their products are available outside of Germany ... Take a look at their website http://www.pattex.de, probably the "Kraftkleber" is the one you are looking for?
Greetings Gunnar
} From: "Quinn, Tim Lee" {tquinn-at-ku.edu} To: "'Microscopy-at-MSA.MIcroscopy.com'" {Microscopy-at-sparc5.microscopy.com}
Hi, You might want to check this paper: 3A critical evaluation of the results of the '92 round robin microanalysis test(EDS & Peels) performed by the Ile de Frande TEMnetwork, in MMM 4, p387-399. (multiple authors) Analysis protocols were discussed in the instance of Olivine. If you want a sample we usedyou should contact J. Ingrin (he is now somewher in Toulouse). Gilles
} } Hallo Folks, } Here's a baffling thing for you to mull over. I'm after some } pointers after scratching my head for a couple of days. Here goes. We } have a JEOL 733 with 4 WD spectrometers. We've the simple task of } analysing some olivine crystals for their major (Si, Mg, Fe) and trace } (Ca, Ni, Mn) elements. This should be a very simple, rudimentary and } stressless thing to do, and normally is. The sad thing is, things aren't } going normally. Standardisation is as simple as possible with as few } standards as possible, and checked rigorously using materials for this } purpose mounted in our standard block. However, when we go to the actual } unknowns, Fe is sytematically about 3 wt % lower than expected for a } stoichiometric olivine assuming the Mg and Si are ok. We can make this } assumption because for an olivine of a specified SiO2 content we would } expect a specified MgO content, and this checks out. For the given FeO } content we would expect lower MgO and SiO2 contents, and this would } simply make the totals worse. I've checked out the hardware and the fact } that the calibration works for unknowns on the standard block suggests } to me that there is no problem with the analytical protocol we're using. } I considered C coating but thought that this is more likely to affect } attenuation of the lower energy X-rays such as Si and Mg. } Has anyone some suggestions on what the cause of this } strange behaviour for a very simple mineral could be? } Thanks, } Malc. } } -- } Dr MP Roberts Phone: [+27](0)46 603 8313 } Dept of Geology Fax: [+27](0)46 622 9715 } Rhodes University Cell: 083 4060 262 (try your luck!) } 6140 Grahamstown e-mail: m.roberts-at-ru.ac.za } SOUTH AFRICA
-- _______________________________________________________ Gilles Hug LEM, UMR 104, ONERA-CNRS, BP72 92322 Chatillon Cedex, France tel : +33 1 46 73 45 42 fax : +33 1 46 73 41 55 mailto:Gilles.Hug-at-onera.fr http://www.onera.fr/lem/anachistr/index.html _______________________________________________________ Office National d'Etudes et de Recherches Aerospatiales ------- & ------ Centre National de la Recherche Scientifique _______________________________________________________
Could some of you please provide me some information regarding where to purchase a 21" or larger low frequency shielded computer monitor? I would like to buy one but having trouble to find a supplier. The monitor will be used to replace the smaller one on our Tecnai TEM. Your help is greatly appreciated.
Thank you, Ping Li
-- Ping Li, Ph.D. Director, Scientific Imaging Suite Department of Biology Dalhousie University Halifax, NS B3H 4J1 Canada
To adhere serial setions together into a ribbon while sectioning, I'v used (with success) a small amount of a product called Tackiwax can be applied to the sides of the blockface at the top and bottom of the trapezoid. I think the reference is in M.A. Hayat's book on EM Techniques for Biological Electron Microscopy.
I ordered a tub (1 lb. container - a lifetime supply for ultramicrotomy) from Fisher Scientific, but other suppliers may be able to get it for you. Here's information off of the label:
Dr. Heather A. Owen, Director Electron Microscope Laboratory Department of Biological Sciences University of Wisconsin - Milwaukee Lapham Hall, P.O. Box 413 Milwaukee, WI 53210 USA
Ladd makes it. It's very nice when using plastic culture dishes. I use the same recipe as for epon 812. Let me know if you need specifics. Mary Gail Engle
At 08:41 AM 8/30/02 -0400, Lesley S. Bechtold wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Mary Gail Engle Sr. Research Laboratory Manager Electron Microscopy & Imaging Facility Health Sciences Research Bldg. 001 University of Kentucky Lexington, KY 40536-0305
The Sony Multiscan E500 (21") and most all of the Multiscan series are shielded.
A better course might be to look into 20" flat panel LCDs. I'm using a 20" RGB+sync unit made in Germany with a NEC LCD display unit. It works quite well. NEC also makes some 18" LCD displays that are very nice. I'm not sure if they make larger ones. The 18" one I have used is the 1850 and is the standard LCD display on the FEI Sirion FEGSEM.
gary
At 04:55 AM 8/30/2002, you wrote:
} Could some of you please provide me some information regarding where to } purchase a 21" or larger low frequency shielded computer monitor? I would } like to buy one but having trouble to find a supplier. The monitor will be } used to replace the smaller one on our Tecnai TEM. Your help is greatly } appreciated. } } Thank you, } Ping Li } } -- } Ping Li, Ph.D. } Director, Scientific Imaging Suite } Department of Biology } Dalhousie University } Halifax, NS B3H 4J1 } Canada } } Tel: 902-494-3309 } Fax: 902-494-3736 } E-mail: Ping.Li-at-Dal.Ca
LX-112 is the EPON replacement sold by LADD. We use is routinely and follow the traditional Luft formulations.
Frank
At 08:41 AM 8/30/02 -0400, Lesley S. Bechtold wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Hi all I am researching salaries. The problem I am having is my job is primarily failure analysis, but I am a technician so most surveys list quality technician and quality engineer. I have responsibilities in both areas. Any help off or online would be most appreciated. 9 years experience.
Apologies for off topic discussion
Robert Fowler Quality Assurance Technician (Failure Analysis) TDK Components USA, Inc. Multilayer Ceramic Capacitor Division 1 TDK Boulevard Peachtree City GA 30269-2051 Telephone: (770) 631-0410 Ext.315 Fax: (770) 487-1460 email: rfowler-at-tdktca.com www.tdk.com
THIS TRANSMISSION IS INTENDED FOR THE SOLE USE OF THE INDIVIDUAL AND ENTITY TO WHOM IT IS ADDRESSED AND MAY CONTAIN PRIVILEGED AND/OR CONFIDENTIAL INFORMATION.
If you are not the intended recipient, be advised that any use, dissemination, distribution or duplication of this transmission is strictly prohibited. If you received this transmission in error, please notify the sender immediately by electronic reply to this transmission or by phone (847-803-6100). Thank you.
LX-112 is a Ladd Research product. It is used in wide variety of projects from EM research to the aerospace industry. Please reply directly with more details on your project, check our web site, http://www.laddresearch.com, or call the number listed below and ask for Dr. Charles Duvic our chemist and you can discuss it with him.
Thank you,
John Arnott
Ladd Research 83 Holly Court Williston, VT 05495
On-line Catalog: http://www.laddresearch.com
tel: 1-802-658-4961(anywhere) or 1-800-451-3406(US) fax: 1-802-660-8859 e-mail: sales-at-laddresearch.com ----- Original Message ----- } From: "Lesley S. Bechtold" {lsb-at-jax.org} To: {microscopy-at-sparc5.microscopy.com} Sent: Friday, August 30, 2002 8:41 AM
Ah....OK. Can you tell us what the basic premise was for doing this? No condemnation, just wondering why you are doing this exercise. As you can imagine, there is a huge range of options, systems and prices.
I'm a cat....curious.
gary g.
At 05:22 AM 8/30/2002, you wrote: } I was not looking for purchase! Just the info } } } ----- Original Message ----- } From: "Gary Gaugler" {gary-at-gaugler.com} } To: "ATC SEM Laboratory" {atcsem-at-earthlink.net} } Cc: "MSA listserver" {Microscopy-at-MSA.Microscopy.Com} } Sent: Thursday, August 29, 2002 9:25 PM } Subject: Re: New SEM opproximate price } } } } Excellent!! what did you recommend for the purchase? } } } } gg } } } } At 04:07 AM 8/27/2002, you wrote: } } } } } I appreciate the information. I think, I've got more than enough. } } } Thank you all very much for comprehensive answers. } } } } } } Pavel } }
Heather A. Owen wrote: ============================================================
To adhere serial setions together into a ribbon while sectioning, I'v used (with success) a small amount of a product called Tackiwax can be applied to the sides of the blockface at the top and bottom of the trapezoid. I think the reference is in M.A. Hayat's book on EM Techniques for Biological Electron Microscopy.
I ordered a tub (1 lb. container - a lifetime supply for ultramicrotomy) from Fisher Scientific, but other suppliers may be able to get it for you. Here's information off of the label:
============================================================== Could someone explain how this product Tackiwax™ apparently a product of Boekel Scientific would differ from a good dental wax, such as on URL www.2spi.com/catalog/knives/cavex-set-up-dental-wax-sh.shtml
which is also used pretty widely in the world for ultramicrotomy applications.
I am not suggesting that this common (but very high quality) dental wax is better for this application, but it is far more readily available from a large number of suppliers (such as one of our many competitors like Ted Pella, Inc.). The Cavex® brand of dental wax, unlike a lot of the dental wax products on the market, is actually approved for use in dentistry in most countries around the world. What is not clear to me is whether soft, medium or hard would be the preferred hardness for this particular application (to adhere serial sections into a ribbon).
The cost to place a small order for a single item, for many customers, can be staggering, so I ask this question because if it is not any different than a good dental wax, such as the Cavex wax, it could keep people in certain countries from placing a small order (because the shipping and other costs of importation may be many times larger than the fob value of the item itself). This is inherently a low cost item and as was pointed out previously, one pack can last virtually a life time.
Disclaimer: SPI Supplies is a major supplier of high quality dental wax for use in microtomy applications worldwide so naturally we would have a vested interest in having customers order this wax from SPI along with their other needed items.
Chuck
============================================
Charles A. Garber, Ph. D. Ph: 1-610-436-5400 President 1-800-2424-SPI SPI SUPPLIES FAX: 1-610-436-5755 PO BOX 656 e-mail:cgarber-at-2spi.com West Chester, PA 19381-0656 USA Cust.Service: spi2spi-at-2spi.com
Look for us! ######################## WWW: http://www.2spi.com ######################## ============================================
I am looking for a replacement part for our poloron sputter/coater. It is a model 0E5000, manufacturing date unknown. The part that is broken is a hollow glass cylinder that has a rubber seal at either end and acts as the sputtering chamber. Any recommendations on a supplier or glass manufacturer is welcomed or other ideas! Thank you in advance.
Wil Kunkel curari-at-asu.edu student of chemistry This email was sent with 100.00% recycled electrons.
The Polaron (check spelling) supplier in the US should be able to get this item for you. If not, that would be a good reason to avoid this brand of coater.
Why did it fail? This seems to me to be a very low failure rate item. The rubber boots do need to be replaced at some interval (like on my Anatech Hummer VII). But having the glass cylinder crack would be really disturbing to me. Did you miss-treat it?
gary g.
At 05:36 PM 8/31/2002, you wrote:
} Dear Listers } } I am looking for a replacement part for our poloron } sputter/coater. It } is a model 0E5000, manufacturing date unknown. The part that is broken is a } hollow glass cylinder that has a rubber seal at either end and acts as the } sputtering chamber. Any recommendations on a supplier or glass } manufacturer is } welcomed or other ideas! Thank you in advance. } } Wil Kunkel } curari-at-asu.edu } student of chemistry } This email was sent with 100.00% recycled electrons.
solar lamps Please look at our web site: {http://www.yt-economy.com/senke.htm} Best regards Zhang Qixing address: nantong road no.71 Yantai China Yantai senke co.ltd tel:86-0535-6675831 fax:86-0535-6675830 post code:264000 email:yt-zqx-at-sohu.com
solar lamps Please look at our web site: {http://www.yt-economy.com/senke.htm} Best regards Zhang Qixing address: nantong road no.71 Yantai China Yantai senke co.ltd tel:86-0535-6675831 fax:86-0535-6675830 post code:264000 email:yt-zqx-at-sohu.com
solar lamps Please look at our web site: {http://www.yt-economy.com/senke.htm} Best regards Zhang Qixing address: nantong road no.71 Yantai China Yantai senke co.ltd tel:86-0535-6675831 fax:86-0535-6675830 post code:264000 email:yt-zqx-at-sohu.com
I recently had the same problem, and I went to the university's glass shop in the chemistry department. Even though the size I needed was a special order item, it still only cost $16, instead of the $120 the sputter-coater company wanted. Yours would cost more, since you would need a groove for the o-ring ground into it, but you'd still save a lot of money. If your department doesn't have a glass shop anyway (a lot of university bean counters have closed the glass shops), then try the big EM facility in mat sci and engineering (I forget the exact department/institute, sorry, but someone on the list will know) -- they have a good-sized machine shop and might be able to make the chamber.
Phil
} Dear Listers } } I am looking for a replacement part for our poloron sputter/coater. It } is a model 0E5000, manufacturing date unknown. The part that is broken is a } hollow glass cylinder that has a rubber seal at either end and acts as the } sputtering chamber. Any recommendations on a supplier or glass } manufacturer is } welcomed or other ideas! Thank you in advance. } } Wil Kunkel } curari-at-asu.edu } student of chemistry } This email was sent with 100.00% recycled electrons.
-- }}}}}}}}}}}}}}}}}{{{{{{{{{{{{{{{{{ Philip Oshel Supervisor, AMFSC and BBPIC microscopy facilities Department of Animal Sciences University of Wisconsin 1675 Observatory Drive Madison, WI 53706 - 1284 voice: (608) 263-4162 fax: (608) 262-5157 (dept. fax)
This email was sent with 100.00% recycled electrons.
On Sun, 1 Sep 2002, Philip Oshel wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Wil, } } I recently had the same problem, and I went to the university's glass } shop in the chemistry department. Even though the size I needed was a } special order item, it still only cost $16, instead of the $120 the } sputter-coater company wanted. } Yours would cost more, since you would need a groove for the o-ring } ground into it, but you'd still save a lot of money. } If your department doesn't have a glass shop anyway (a lot of } university bean counters have closed the glass shops), then try the } big EM facility in mat sci and engineering (I forget the exact } department/institute, sorry, but someone on the list will know) -- } they have a good-sized machine shop and might be able to make the } chamber. } } Phil } } } Dear Listers } } } } I am looking for a replacement part for our poloron sputter/coater. It } } is a model 0E5000, manufacturing date unknown. The part that is broken is a } } hollow glass cylinder that has a rubber seal at either end and acts as the } } sputtering chamber. Any recommendations on a supplier or glass } } manufacturer is } } welcomed or other ideas! Thank you in advance. } } } } Wil Kunkel } } curari-at-asu.edu } } student of chemistry } } This email was sent with 100.00% recycled electrons. } } -- } }}}}}}}}}}}}}}}}}{{{{{{{{{{{{{{{{{ } Philip Oshel } Supervisor, AMFSC and BBPIC microscopy facilities } Department of Animal Sciences } University of Wisconsin } 1675 Observatory Drive } Madison, WI 53706 - 1284 } voice: (608) 263-4162 } fax: (608) 262-5157 (dept. fax) } }
I also use Sony Multiscan sfII shielded monitors on PCs and Macs.
Look at Emission/EMI and ELF/VLF specs for prospective units.
This is their new 21" monitor: http://www.sonystyle.com/home/item.jsp?hierc=9683&itemid=8241
This is their 24" monitor (100 pounds--heavy!!): http://www.sonystyle.com/home/item.jsp?hierc=9683&catid=9710&itemid=6971
These are shielded.
NEC makes good monitors too. Many of them are also shielded. Check before you buy.
gary
At 04:55 AM 8/30/2002, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
A faculty member needs to produce some extremely high resolution 24 x 35 mm negatives or masks to demonstrate the diffraction phenomenon and FFT. He has generated around 24 PostScript files that consist of a "unit cell" (such as an Escher figure) that is repeated numerous times to mimic a crystalline lattice. The goal is to project a laser through the negative masks and generate diffraction patterns as part of the demonstration.
We have attempted to generate hi res 35 mm negs by means of a LaserGraphics 8,000 line film recorder but the resolution is inadequate. He needs the equivalent of 16,000 x 24,000 pixels in the 24 x 35 mm area. This is about 17,000 ppi!
Any suggestions? Any other practical ways to produce these masks?
I had considered micro-lithography but do not have access to the technology.
Many thanks,
John B.
############################################################## John J. Bozzola, Ph.D., Director I.M.A.G.E. (Integrated Microscopy & Graphics Expertise) 750 Communications Drive - MC 4402 Southern Illinois University Carbondale, IL 62901 U.S.A. Phone: 618-453-3730 Fax: 618-453-2665 Email: bozzola-at-siu.edu Web: http://www.siu.edu/~image/ ##############################################################
John Sounds too demanding for a demonstration. Is it not possible to get the same value from the demonstration by using a less complex image, with lower definition and fewer repeats? Chris
----- Original Message ----- } From: "John J. Bozzola" {bozzola-at-siu.edu} To: {Microscopy-at-sparc5.microscopy.com} Sent: Monday, September 02, 2002 11:00 PM
} } Dear colleagues and friends, } } } } please find below the ascii version of the first Call for Paper of the } } } conference MIRAGE'2003; please feel free to distribute it and to } advertise. } } } } The website of the conference is http://telin.rug.ac.be/mirage2003 } } } } Looking forward to meeting you in Rocquencourt, } } } } Jacques Blanc-Talon and Andre Gagalowicz } } } } } --- } } } } MIRAGE 2003 } } } } Call for Papers } } } } Computer Vision / Computer Graphics } } Collaboration for } } Model-based Imaging, } } Rendering, } } image Analysis and } } Graphical special Effects } } } } 10-12 March 2003 } } INRIA Rocquencourt, France } } } } MIRAGE 2003 is designed as a very peculiar conference in the field of } } } Information Technology: it is dedicated to computer vision and } } } computer graphics collaboration studied as a tool for the production } } } of mirages of the reality. In the domain of computer vision, this } } } collaboration may take the form of model-based approaches with } } } feedback, as models are essential to process, analyze, understand and } } } generate complex still and animated images in a stable manner. Such } } } models must be comprehensive and their parameters updated according to } } } the difference between the expectation (real image) and the } } } synthesized results. In the computer graphics domain, a special } } } emphasis will be set upon techniques using real images as input for } } } realistic rendering, visualization and special effects. } } } } MIRAGE 2003 is going to be an international conference where authors } } } are encouraged to submit papers on theoretical, computational, } } } experimental and industrial aspects of model-based image analysis and } } } synthesis. MIRAGE'2003 will be held in the new conference room of the } } } INRIA Rocquencourt research centre on March 10-12, 2003. } } } } Topics include (but are not limited to) } } } } * Model-based imaging and analysis } } * Model-based vision approaches } } * Model-based indexing and database retrieval } } * Model-based object tracking in image sequences } } * Image-based rendering and inverse rendering techniques } } * New trends in model-based (and intrinsic) video compression } techniques } } * Virtual and augmented reality } } * Generation of special effects } } * Model-based evaluation of computer vision techniques, Image } quality } } * Applications: } } o Human-computer interaction, haptics } } o Virtual prototyping } } o Post-production, computer animation } } o Multimedia applications (including face and gesture } recognition), } } multimedia databases } } o Military applications } } o Medical and biomedical applications } } o Applications of fractals and multifractals } } } } Venue } } } } The Symposium will take place within the INRIA Rocquencourt research } } } centre which can be easily reached by car, by train or by bus, either } } } by taking public transportations or the free INRIA facilities. The } } } different routes are fully detailed on the INRIA special webpage. } } } } Paper submission and review process } } } } Prospective authors should prepare a full paper and submit it } } } electronically. The paper should consist of 5-10 pages in A4 format } } } with 11 pt font and should conform to the style guidelines outlined on } } } the MIRAGE 2003 website. LaTeX style sheets, MSWord templates and more } } } detailed information on the submission process can be found on the } } } MIRAGE 2003 website. } } } } All submissions will be reviewed by at least 2 members of the Program } } } Committee; additional reviewers will be consulted if necessary. The } } } papers should provide sufficient background information and should } } } clearly indicate the original contribution. They should state and } } } discuss the main results and provide adequate references. } } } } Confererence proceedings } } } } Accepted papers will be published in the CD-Rom conference proceedings } } } in pdf-format. Authors will be encouraged to include additional } } } multimedia content like sound files, demo's and video sequences, } } } subject to space availability. Authors wishing to take advantage of } } } this possibility should contact the Steering Committee for additional } } } instructions. } } } } Important deadlines } } } } November 12, 2002 Full paper submission } } December 20, 2002 Notification of acceptance } } February 10, 2003 Camera-ready papers due } } January 6, 2003 Early registration deadline } } February 10, 2003 Late registration deadline } } 10-12 March 2003 MIRAGE 2003 } } } } Registration } } } } Registration will be available online at the beginning of } } } 2003. However, due to security policy, the number of seats is strictly } } } limited: thus, early registration is strongly recommended. } } } } Conference Chair } } } } Jacques Blanc-Talon, CTA, Arcueil, France } } Andre Gagalowicz, INRIA, Rocquencourt, France } } } } Steering Committee } } } } Jacques Blanc-Talon, CTA, Arcueil, France } } Andre Gagalowicz, INRIA Rocquencourt, France } } Philippe Gérard, INRIA Rocquencourt, France } } Wilfried Philips, Ghent University, Gent, Belgium } } Dominique Potherat INRIA Rocquencourt, France } } } } Honorary Chair } } } } Hojjat Adeli, Ohio State University, Colombus, USA } } } } Program committee } } } } Ruzena Bajcsy, UC Berkeley, USA } } Philippe Bolon, ESIA, Annecy, France } } Mike Brooks, University of Adelaide, Australia } } Knut Conradsen, IMM, Denmark Technical University, Denmark } } Kostas Daniilidis, U-Penn, USA } } Charles R. Dyer, University of Wisconsin-Madison, USA } } Andrew Glassner, Coyote Wind, Seattle, USA } } Cedric Guiard, Duran Duboi, France } } Adrian Hilton, University of Surrey, UK } } David Hogg, University of Leeds, UK } } Xiaoyi Jiang, Technical University of Berlin, Germany } } Denis Laurendeau, Laval University, Quebec City, Canada } } Franz Leberl, Graz University of Technology, Austria } } Ales Leonardis, Ljubljana University, Slovenia } } Vittorio Murino, Verone University, Italy } } Jean-Claude Paul, LORIA, France } } Hichem Sahli, Vrije Universiteit Brussel, Belgium } } Mubarak Shah, University of Central Florida, USA } } Gilles Simon, LORIA, Vandoeuvre-les-Nancy, France } } Franck Solina, Ljubljana University, Slovenia } } Seah Hock Soon, NTU, Singapore } } Geoff West, Curtin University, Australia } } Geoff Wyvill, University of Otago, New Zealand } } Luc Van Gool, ESAT, Leuven, Belgium (ETH, Zurich, Switzerland) } } } } } -------------------------------------------------------------------------- -- } } } } } best regards! } } André Gagalowicz } }
Hello all ! Maybe somebody knows how to analyse samples of clinoptilolite containing strontium on EDX detector. Strontium and Silicon have both peak in one line. Please help me. This is my doc work.
I suppose you need the small periodicity to achieve larger "bragg angles" so you can show the diffraction pattern. If you make your pattern bigger (fewer dots per inch), your diffraction angles are reduced, but could you perhaps make up for that by using a longer "camera length", i.e., project the results on a screen further away, or use some optics? Perhaps you could use an old slide projector in some inventive fashion.
By the way, what resolution is an 8000 line film recorder? 24 mm / 8000 lines = 3 microns per line or about 8000 dpi?
mike
Michael Bode, Ph.D. Soft Imaging System Corp. 12596 West Bayaud Avenue Suite 300 Lakewood, CO 80228 =================================== phone: (888) FIND SIS (303) 234-9270 fax: (303) 234-9271 email: mailto:info-at-soft-imaging.com web: http://www.soft-imaging.com ===================================
-----Original Message----- } From: John J. Bozzola [mailto:bozzola-at-siu.edu] Sent: Monday, September 02, 2002 4:01 PM To: Microscopy-at-sparc5.microscopy.com
A faculty member needs to produce some extremely high resolution 24 x 35 mm negatives or masks to demonstrate the diffraction phenomenon and FFT. He has generated around 24 PostScript files that consist of a "unit cell" (such as an Escher figure) that is repeated numerous times to mimic a crystalline lattice. The goal is to project a laser through the negative masks and generate diffraction patterns as part of the demonstration.
We have attempted to generate hi res 35 mm negs by means of a LaserGraphics 8,000 line film recorder but the resolution is inadequate. He needs the equivalent of 16,000 x 24,000 pixels in the 24 x 35 mm area. This is about 17,000 ppi!
Any suggestions? Any other practical ways to produce these masks?
I had considered micro-lithography but do not have access to the technology.
Many thanks,
John B.
############################################################## John J. Bozzola, Ph.D., Director I.M.A.G.E. (Integrated Microscopy & Graphics Expertise) 750 Communications Drive - MC 4402 Southern Illinois University Carbondale, IL 62901 U.S.A. Phone: 618-453-3730 Fax: 618-453-2665 Email: bozzola-at-siu.edu Web: http://www.siu.edu/~image/ ##############################################################
A couple of details in your post raised some flags, though I'm not sure of the exact numbers below:
} He needs the equivalent of 16,000 x 24,000 pixels in the 24 x 35 mm area
- Though it's still a topic of debate, I believe the estimate for "pixel equivalent" of a fine-grained 35mm film shot with a high quality lens is around 20 million total pixels (~4000 dpi), which you've already exceeded by quite a bit with the 8,000 line LFR. Even if my memory on this issue is off by millions of pixels, I'm quite sure there is no way 35mm film could support 16,000 x 24,000 pixels.
As far as I can tell, you could get close by upgrading your Lasergraphics film recorder to their 16,000 line "Mark VI" model (16384 x 13448 addressable pixels), and use the 4" x 5" (~ 16k x 20k pixel equivalent film) camera back. You may want to see if some other manufacturer has a film recorder with more than 16,000 lines if you truly need 16,000 x 24,000 pixels. We have the same 8,000 line LFR in our lab, so I can't give any insight on what the upgrade might cost.
I have no knowledge of or experience with producing masks, so I don't know if 4" x 5" is a viable option.
Kevin Frischmann Microscopy & Imaging Facility American Museum of Natural History Central Park West at 79th Street New York, NY 10024-5192 USA
At 05:00 PM 9/2/02 -0500, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
As a follow on, at 17,000 DPI, are you approaching (or passing) the resolution of the 35mm film?
Does anybody know the size of the Silver Halide Molecules on the film?
John W. Raffensperger, Jr. IS Manager Helwig Carbon Products, Inc.
-----Original Message----- } From: Chris Jeffree [mailto:c.jeffree-at-ed.ac.uk] Sent: Tuesday, September 03, 2002 2:59 AM To: John J. Bozzola Cc: microscopy-at-sparc5.microscopy.com
Aperio's scanner will do this easily - see http://www.aperio.com
-----Original Message----- } From: Kevin Frischmann [mailto:kfrisch-at-amnh.org] Sent: Tuesday, September 03, 2002 12:05 PM To: Microscopy-at-sparc5.microscopy.com
John,
A couple of details in your post raised some flags, though I'm not sure of the exact numbers below:
} He needs the equivalent of 16,000 x 24,000 pixels in the 24 x 35 mm area
- Though it's still a topic of debate, I believe the estimate for "pixel equivalent" of a fine-grained 35mm film shot with a high quality lens is around 20 million total pixels (~4000 dpi), which you've already exceeded by quite a bit with the 8,000 line LFR. Even if my memory on this issue is off by millions of pixels, I'm quite sure there is no way 35mm film could support 16,000 x 24,000 pixels.
As far as I can tell, you could get close by upgrading your Lasergraphics film recorder to their 16,000 line "Mark VI" model (16384 x 13448 addressable pixels), and use the 4" x 5" (~ 16k x 20k pixel equivalent film) camera back. You may want to see if some other manufacturer has a film recorder with more than 16,000 lines if you truly need 16,000 x 24,000 pixels. We have the same 8,000 line LFR in our lab, so I can't give any insight on what the upgrade might cost.
I have no knowledge of or experience with producing masks, so I don't know if 4" x 5" is a viable option.
Kevin Frischmann Microscopy & Imaging Facility American Museum of Natural History Central Park West at 79th Street New York, NY 10024-5192 USA
At 05:00 PM 9/2/02 -0500, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Sorvall MT-2B Ultramicrotome for sale. Includes manual and accessories. If interested, contact me via e-mail.
Martin L. Katz, PH.D. University of Missouri Ophthalmology, Genetics, Pathobiology & Molecular Biology Mason Eye Institute One Hospital Drive Columbia, MO 65212 (573) 882-8480 FAX (573) 884-4100 katzm-at-health.missouri.edu
Randy Tindall EM Specialist Electron Microscopy Core Facility W122 Veterinary Medicine University of Missouri Columbia, MO 65211 Tel: (573) 882-8304 Fax: (573) 884-5414 Email: tindallr-at-missouri.edu Web: http://www.biotech.missouri.edu/emc/
Try looking at 14.164 Kev, should be a K line down there.
William Giles Senior Electron Microscopist Metallography Lab Coordinator P.O. Box 2128 Henderson, Nevada 89009 (702) 566-4436 (702) 564-9038 (Fax) Bill.Giles-at-timet.com
RE: Hello all ! Maybe somebody knows how to analyse samples of clinoptilolite containing strontium on EDX detector. Strontium and Silicon have both peak in one line. Please help me. This is my doc work.
I missed on this one too. The fellow is looking for making a slide, not scanning one. I think the highest resolution is probably via a microcircuit stepper mask (5"x5" chrome on quartz). The image size can be just about anything up to the size of the plate. Price is big too.
gary
At 11:31 AM 9/3/2002, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Photolithography, as is used in semiconductors, would certainly give you the spatial resolution you desire but is an expensive proposition for a demonstraion.
Peter Tomic Anadigics, Inc.
-----Original Message----- } From: John J. Bozzola [mailto:bozzola-at-siu.edu] Sent: Monday, September 02, 2002 6:01 PM To: Microscopy-at-sparc5.microscopy.com
A faculty member needs to produce some extremely high resolution 24 x 35 mm negatives or masks to demonstrate the diffraction phenomenon and FFT. He has generated around 24 PostScript files that consist of a "unit cell" (such as an Escher figure) that is repeated numerous times to mimic a crystalline lattice. The goal is to project a laser through the negative masks and generate diffraction patterns as part of the demonstration.
We have attempted to generate hi res 35 mm negs by means of a LaserGraphics 8,000 line film recorder but the resolution is inadequate. He needs the equivalent of 16,000 x 24,000 pixels in the 24 x 35 mm area. This is about 17,000 ppi!
Any suggestions? Any other practical ways to produce these masks?
I had considered micro-lithography but do not have access to the technology.
Many thanks,
John B.
############################################################## John J. Bozzola, Ph.D., Director I.M.A.G.E. (Integrated Microscopy & Graphics Expertise) 750 Communications Drive - MC 4402 Southern Illinois University Carbondale, IL 62901 U.S.A. Phone: 618-453-3730 Fax: 618-453-2665 Email: bozzola-at-siu.edu Web: http://www.siu.edu/~image/ ##############################################################
there is no simple answer to your question, as the speed of the film has a big influence on the resolution (faster films use larger grains). Also development will change the number of pixels. I did a quick search on the internet and I found 2 sites with specific answers. I have included excerpts below, there is more information on those sites.
It seems, the answer is somewhere between 10 Million and 20 Million pixels, but that is of course only a qualitative answer. A full answer would have to take into account the modulation transfer function, dynamic range, etc. The second link below goes into that a bit. For example, the author says that a certain film can resolve 3500 line pairs (7000 pixels) over the width of the film (35mm), but that only means, that at that resolution one can distinguish a white line from a black line with some accuracy. In digital parlance that would probably mean a dynamic range of 1 bit (black or white). If you want to have a better dynamic range (to distinguish for example black from dark gray), you would have to look at larger areas, thus reducing the resolution.
mike
Michael Bode, Ph.D. Soft Imaging System Corp. 12596 West Bayaud Avenue Suite 300 Lakewood, CO 80228 =================================== phone: (888) FIND SIS (303) 234-9270 fax: (303) 234-9271 email: mailto:info-at-soft-imaging.com web: http://www.soft-imaging.com ===================================
http://pic.templetons.com/brad/photo/pixels.html How many pixels are there in a frame of 35mm film?
(an FAQ on digital photography)
This is a somewhat controversial question, and there are many possible answers. Film is an analog medium, so it doesn't have "pixels" per se, though film scanners have pixels and a specific resolution.
Today the one thing most people agree on is that it's a lot more than any current consumer digital camera. The debate is about how much resolution the digitals will have to reach to start matching the film.
The very short answer is that there are around 20 million "quality" pixels in a top-quality 35mm shot. That's a shot with a tripod, mirror-up, with a top-rate lens and the finest-grained film, in decent light. 12 million are more typical for "good" shots. There may be as few as 4 million "quality" pixels in a handheld shot with a point-and-shoot camera or camera with a poor lens. And of course if focus is poor, or light is poor, or the camera was not held steady, the number will drop down below the 1-2 million pixels of the modern consumer digicam. Of course, one can have a bad shot with a digital camera too, not using all its resolving ability. However, few pick their gear with the plan of shooting badly. ..
http://www.bytesmiths.com/Services/scanning.html The dimensions of a digital image are often confused with its resolution, but it is actually a count of pixels (width by height) that is independent of any unit of measure. A highest-quality, 35mm film scan will have dimensions of about 3600x2400 pixels. ..
-----Original Message----- } From: John W. Raffensperger, Jr. [mailto:johnr-at-helwigcp.com] Sent: Tuesday, September 03, 2002 11:51 AM To: microscopy-at-sparc5.microscopy.com
John;
As a follow on, at 17,000 DPI, are you approaching (or passing) the resolution of the 35mm film?
Does anybody know the size of the Silver Halide Molecules on the film?
John W. Raffensperger, Jr. IS Manager Helwig Carbon Products, Inc.
-----Original Message----- } From: Chris Jeffree [mailto:c.jeffree-at-ed.ac.uk] Sent: Tuesday, September 03, 2002 2:59 AM To: John J. Bozzola Cc: microscopy-at-sparc5.microscopy.com
http://www.themonitoroutlet.com has every monitor known to man.
John Mardinly Intel
-----Original Message----- } From: Ping Li [mailto:pli-at-dal.ca] Sent: Friday, August 30, 2002 4:56 AM To: Microscopy-at-sparc5.microscopy.com
Could some of you please provide me some information regarding where to purchase a 21" or larger low frequency shielded computer monitor? I would like to buy one but having trouble to find a supplier. The monitor will be used to replace the smaller one on our Tecnai TEM. Your help is greatly appreciated.
Thank you, Ping Li
-- Ping Li, Ph.D. Director, Scientific Imaging Suite Department of Biology Dalhousie University Halifax, NS B3H 4J1 Canada
} } } Hello all ! } Maybe somebody knows how to analyse samples of clinoptilolite } containing strontium on EDX detector. Strontium and Silicon have both } peak in one line. Please help me. This is my doc work. } } }
WDS would be better, but if you just can't get to it, maybe you could bang the accelerating voltage up to 25 or even 30 kV and analyse on the Sr Ka line at about 15 kV. I haven't done it for Sr, but I did use 25 kV for Mo Ka to avoid SKa, worked OK.
good luck
rtch
Ritchie Sims Phone : 64 9 3737599 ext 7713 Department of Geology Fax : 64 9 3737435 The University of Auckland email : r.sims-at-auckland.ac.nz Private Bag 92019 Auckland New Zealand
I would appreciate some advice on low temperature embedding in the Leica EM AFS freeze substitution unit using LR gold. Sorry, since I am a beginner (concerning TEM) some of my questions might sound a little odd.
My aim is to do immunogold labelling, mainly on cell walls, with sections from Arabidopsis roots. The plan is to high pressure freeze Arabidopsis roots, freeze substitute them, and embed them in LR gold at low temperature (-25 degrees).
At the moment I am running a few tests before I start the real experiment. And I am having trouble with the LR gold embedding.
This is what I tried so far: I followed the protocol for "FS and low temperature embedding in LEICA-capsules" from the AFS handbook (5.2, p.35). I was using LR gold + 0.5% Benzil (w/v) as embedding medium. I started polymerisation at -25 degrees with the UV lamp (Leica EM UV). After 24h the resin was not yet solidified, only the bottom half of the capsules looked like it was solid.
My questions: Does anybody have experience with low temperature embedding using LR gold in the Leica EM AFS? Any ideas how long UV-polymerisation might take? (24h was the information I got from the supplier for the LR gold). Or is there an easier way of getting my specimens embedded, preferably in the Leica EM AFS?
Thanks a lot for your help,
Regina
------------------------------------------------------------------- Dr. Regina Himmelspach Plant Cell Biology Group Research School of Biological Sciences The Australian National University GPO Box 475 Canberra ACT 2601 Australia
Interesting question, particularly now when EMs are found in such a wide range of applications. I'll share what seems to work for me, although I make no claim that this is the way training should be done.
I've trained quite a number of operators. I want them to first know those things that can cause damage (i.e. - don't touch that TEM phosphor screen). The instruments are frightening at first, and having some limits will actually be comforting to them - they can focus on those things and relax with the rest. Don't overload them with don't do's - just cover the things that may cause expensive or time consuming damage.
My own desire is always to have the operator understand the physics behind the instrument, and I always explain things in those terms. Knowing that increasing the condenser current in an EM decreases the spot size gives you little. Knowing that it reduces the chromatic spread or aberration of the beam, and how, gives a broader understanding of the mechanism and the result. While the distinction may not be terribly helpful in normal use it gives them something that may help in the unusual circumstances.
That's what you really have to plan for in training, the unusual circumstances. I've seen a number of customers in recent years who have absolutely no knowledge of the instruments. 'Checklist operators' I call them, and that's literally how they work. The person who bought the instrument is long gone from the company, but he left a checklist for the operation of the instrument that has been faithfully followed since. It's a minor annoyance for me since I get service calls when someone accidentally touches the wrong knob or they get a different type of sample where the standard setup won't work. That stuff is minor, though, and truly the extreme.
These are some really great tools, kind of like a hammer. When you need to drive a nail, nothing works better. When you need to look at something with a magnification greater than a light microscope, nothing beats EM. But they are getting more trivialized as more production use is made of them. These are more than a simple tool - they are the most sophisticated equipment you'll find in a lab. Their proper and useful use requires operators who know their limitations as well as their operation. One of the things I always want to ensure is that the operators, if not the management, understand what to really expect regarding the application and interpretation of EMs.
All of this is in a lecture setting - I don't expect them to consciously remember what I've told them over the hour or two it takes. Rather, I hope that when they need it, they'll connect the dots with something I said and figure out for themselves what's needed.
Then it's on to hands on training. This is generally very short - I can teach someone to take a usable picture in five minutes. A little more time looking over their shoulder while they look around. But then it's time to get out.
The next two steps are the most important, bar none. Give them time to play and learn for themselves the questions to ask, and follow up.
It takes time to get comfortable operating an instrument like these. It takes time to play around with different samples and conditions. It takes time to discover the questions you need help answering. The potential operators simply have to spend a lot of time playing, not working, with an EM to become good operators. If they are required to immediately start working, you may get a good 'checklist operator' for the samples you regularly run, and that may be enough. But if you want someone who really understands the instrument, its use and its limitations, you have to encourage them to explore the envelope.
Follow up - you have to follow up. Don't do it too quick, give them some time to play. You have to take the initiative to query the potential operator regarding the questions they have accumulated (suggest they write them down) and the samples and conditions they have explored. This is your chance to add details and refine their knowledge of the use and limitations of the instrument. They're starting to learn the questions to ask - they need to know that there is someone there to help with these problems. If you're not there, then they will come to their own conclusions. Sometimes they might be right, sometimes they might be wrong - in either case, if you don't follow up you'll be missing out on your best possibility to really train.
Have fun!
Allen R. Sampson Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174
On Tuesday, September 03, 2002 11:35 AM, Lois Anderson [SMTP:landers-at-jhmi.edu] wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Has anyone ever trained an inexperienced EM tech and if so do you have } any suggested tactics? }
Does anyone know of any companies out there that rebuild LaB6 cathodes? Has anyone had good/bad experiences with them? Vendors, please reply off-list....
Frank Thomas Geological Survey of Canada (Atlantic) Bedford Institute of Oceanography Dartmouth, Nova Scotia Canada
-----Original Message----- } From: Gary Gaugler [mailto:gary-at-gaugler.com] Sent: Tuesday, September 03, 2002 5:48 PM To: microbill-at-mohawk.net Cc: MSA listserver
I missed on this one too. The fellow is looking for making a slide, not scanning one. I think the highest resolution is probably via a microcircuit stepper mask (5"x5" chrome on quartz). The image size can be just about anything up to the size of the plate. Price is big too.
gary
At 11:31 AM 9/3/2002, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
It's true that Si & Sr overlap at ~ 1.8 KeV. The Sr major La1 line is at 1.806 KeV and the Si Ka1 major line is at 1.739 KeV. However, Sr is a much more complex atom and has a Ka1 major line at 14.164 KeV as Bill Giles mentioned below. Sr should be easily discernable from Si. Of course you will have to have an incident electron energy of about 1.5 to 2X of the Sr Ka1 energy to see it. I assume you can run your survey at 25 to 30 KeV?
Peter Tomic Anadigics, Inc.
-----Original Message----- } From: Giles, Bill [mailto:William.Giles-at-timet.com] Sent: Tuesday, September 03, 2002 4:29 PM To: 'Microscopy-at-MSA.Microscopy.Com'
Try looking at 14.164 Kev, should be a K line down there.
William Giles Senior Electron Microscopist Metallography Lab Coordinator P.O. Box 2128 Henderson, Nevada 89009 (702) 566-4436 (702) 564-9038 (Fax) Bill.Giles-at-timet.com
RE: Hello all ! Maybe somebody knows how to analyse samples of clinoptilolite containing strontium on EDX detector. Strontium and Silicon have both peak in one line. Please help me. This is my doc work.
are you talking about training from scratch? ie fixation, sectioning etc? if so there is a long row to hoe. the best bet is always start from the somplest to the more complicated, and train in the order they would normaly do things, such as embedding then triming then sections (thicks then thins) staining then finaly to the scope. always include the theory in with the practical. depending on how motivated the person is and how big an ego they have traing could take anywhere from a week to the person never getting it. when i learned Em it was in a class room setting with the prof showing us once how to do things then for the rest of the semester we were on our own, lots of students droped the course. the few that stuck it out became very good and advanced techs. this is not i repeat not the recommended method of training someone. i still have thoughts of how to get even with the prof. john
} } Has anyone ever trained an inexperienced EM tech and if so do you have } any suggested tactics?
*************** I have taught and EM course a number of times and have trained technicians who had no background. Slow and steady wins the race. I have found that taking the time to explain WHY things are done, and WHAT the aims of each procedure are is very helpful. You can just make people memorize techniques, but without understanding they will always be automatons and won't be able to deal with anything unexpected. So, don't just give them a dehydration protocol, explain why you need to extract the water, etc. Also, take it one step at a time, don't try to teach the person everything, tissue to grid, in one fell swoop.
The good ting is that you can teach this person how to do things the way you like, and they don't have any conflicting ideas.
Good luck, Lee -- Leona Cohen-Gould, M.S. Sr. Staff Associate Director, Electron Microscopy Core Facility Manager, Optical Microscopy Core Facility Joan & Sanford I. Weill Medical College of Cornell University voice (212)746-6146 fax (212)746-8175
Allen touched on a significant point. I haven't had the pleasure of working with an EM, but the concept applies to other technology as well.
As the "front ends" of technological devices get "better" and easier to use, it becomes easier and easier to "get results". Just about anyone can get some type of reading/image/measurement from a piece of modern equipment.
Getting a result, and getting a MEANINGFUL result are two very different things. Without a background understanding of the fundamental concepts involved in how a particular device/technology works, the operator is at risk of getting a result that may appear meaningful, but is beyond the capabilities of the equipment (and/or sample preparation techniques).
An example I can directly relate to is on a 3-D Coordinate Measuring Machine. In the "old days", the interfaces were crude, and you needed to have a pretty thorough understanding of 3-D geometry just to get a reading. Now, with the graphical interfaces, just about anyone can walk up, use the joystick and touch the part in a few places, and get a reading. But without the fundamental understanding, they may not have set a meaningful reference plane and axis. As a result, they did indeed get a result, but a meaningless one.
John W. Raffensperger, Jr. IS Manager Helwig Carbon Products, Inc.
-----Original Message----- } From: Allen Sampson [mailto:ars-at-sem.com] Sent: Wednesday, September 04, 2002 1:40 AM To: 'Lois Anderson'; microscopy-at-sparc5.microscopy.com
Dear Wil,
We are the authorized Polaron dealer in the U.S. Please contact us at ebs-at-ebsciences.com or by phone on (800) 992-9037 and we will be happy to help you with any parts, service or new instrument requirements you have.
Michael R. Nesta General Manager Energy Beam Sciences, Inc. Agawam, MA USA Tel: (413) 786-9322 "Adding Brilliance to Your Vision"
-----Original Message----- } From: "curari-at-asu.edu"-at-sparc5.microscopy.com [mailto:"curari-at-asu.edu"-at-sparc5.microscopy.com] Sent: Saturday, August 31, 2002 8:36 PM To: Microscopy
Dear Listers
I am looking for a replacement part for our poloron sputter/coater. It is a model 0E5000, manufacturing date unknown. The part that is broken is a hollow glass cylinder that has a rubber seal at either end and acts as the sputtering chamber. Any recommendations on a supplier or glass manufacturer is welcomed or other ideas! Thank you in advance.
Wil Kunkel curari-at-asu.edu student of chemistry This email was sent with 100.00% recycled electrons.
We are the authorized Polaron dealer in the U.S. Please contact us at ebs-at-ebsciences.com or by phone on (800) 992-9037 and we will be happy to help you with any parts, service or new instrument requirements you have.
Michael R. Nesta General Manager Energy Beam Sciences, Inc. Agawam, MA USA Tel: (413) 786-9322 "Adding Brilliance to Your Vision"
-----Original Message----- } From: "curari-at-asu.edu"-at-sparc5.microscopy.com [mailto:"curari-at-asu.edu"-at-sparc5.microscopy.com] Sent: Saturday, August 31, 2002 8:36 PM To: Microscopy
Dear Listers
I am looking for a replacement part for our poloron sputter/coater. It is a model 0E5000, manufacturing date unknown. The part that is broken is a hollow glass cylinder that has a rubber seal at either end and acts as the sputtering chamber. Any recommendations on a supplier or glass manufacturer is welcomed or other ideas! Thank you in advance.
Wil Kunkel curari-at-asu.edu student of chemistry This email was sent with 100.00% recycled electrons.
We train 8-16 students how to use the SEM and TEM a year here. In general 99% of them have no clue where to begin. I do follow pretty much a line similar to what Allan Sampson talked about. BUT I don't go deep into the physics of the system until they get out of the intro class and into the advanced class. We have a 3 check out system. First one is 2 hours with 2 students and me. Sample loading - what you can do to screw it up - "review the checklist" - and generally go over the basics - sample moving, mag, focus, collecting an image. The second checkout is 2 hours with 1 student. I sit down and spend 15 minutes going over everything with them and then leave them there with instructions to collect 3-4 images of what ever they want (sample already in). I check on them through the 2 hours - answer questions, offer pointers, generally lightly supervise them. The final session is basically instruction free. A test if you will. One so that they can demonstrate to me that they understand enough about what they are doing so as not to break anything and then they get keys to the rooms. Instruction is carried out in the classes on specific areas with demonstrations and lab write-ups. But even for student researchers that are not enrolled in the class, they receive very similar instruction, but tailored more to their individual project. The emphasis is always - ask questions! Make sure they realize that if they are stuck then need to ask questions rather than waste an hour or more of beam time trying to figure something out themselves.
The standard checklist protocol is critical, but it can't be a substitute for hands on instructions. Scare them but not enough that they are afraid to touch stuff, reassure them so they have confidence but not enough that they are more likely to break something. Emphasize that if they DO do something resulting in a failure or a problem that they document exactly what they did leading up to the problem and that they won't get in trouble and that it is essential that what happened leading up to the problem be fully disclosed so that the problem can be fixed as fast as possible.
Hope this helps - it works for us here.
Geoff Williams Microscopy Facility Supervisor
Checkout the new Biology Department Microscopy Facility web page. Version 1 is now On-Line: www.cst.cmich.edu/users/willi1gl/BDMF/BDMF.htm
} -----Original Message----- } From: Lois Anderson [mailto:landers-at-jhmi.edu] } Sent: Tuesday, September 03, 2002 2:35 PM } To: microscopy-at-sparc5.microscopy.com } Subject: trainee } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Has anyone ever trained an inexperienced EM tech and if so do you have } any suggested tactics?
In training or help to train dozens of people over the years, I have run across one phenomenon that has always puzzled me. I first noticed this when showing people how to do specimen exchanges in TEM's in which a premature turning of the specimen arm before sufficient pumping on the airlock causes the high-voltage to shut down. Sometimes it would take around 20 minutes to get the scope back on line, and there can actually be introduction of a bit of oil into the column.
Needless to say, I wanted to warn trainees about this, so I first started telling them something like "Insert the specimen arm, BUT DO NOT TURN IT UNTIL....." Almost invariably, this resulted in exactly what I wanted to avoid, usually the first or second time I wasn't there to watch. Finally, I switched to saying "Insert the specimen arm and push it into place with the flat of your hand, then after the light goes out, turn it clockwise". That seems to work.
The point is, I guess, that in training people about things that can potentially damage equipment, I have found it best NOT to say "Don't ever do this!" It works much better (for me) to say "Do it like this." and demonstrate a way that minimizes the chance of an accident. Later on, after the habit has been established, I can explain the reasons without causing bad things to happen.
Has anyone else experienced this? Is this Edgar Allen Poe's "Imp of the Perverse" or just, gulp, me?
Randy
Randy Tindall EM Specialist Electron Microscopy Core Facility W122 Veterinary Medicine University of Missouri Columbia, MO 65211 Tel: (573) 882-8304 Fax: (573) 884-5414 Email: tindallr-at-missouri.edu Web: http://www.biotech.missouri.edu/emc/
Is it too early to inquire as to the status of mailings of the proceedings? If not, could someone direct me to the appropriate individual or committee responsible for the mailings so that I could determine when I could expect mine to arrive. I seem to remember that last year there were many postings to the list on the subject of late deliveries. I haven't seen any this year, so maybe I'm the exception. Please disregard this note if my copy is already in my mailbox.
Randy, This is called Neuro-Linguistic Programming (NLP) by some. http://www.nlptraining.com/index.asp
Disclaimer: The above link is for your information only.
} From: "Tindall, Randy D." {TindallR-at-missouri.edu} } To: {microscopy-at-sparc5.microscopy.com} } X-OriginalArrivalTime: 04 Sep 2002 17:43:49.0465 (UTC) } } } In training or help to train dozens of people over the years, I have run } across one phenomenon that has always puzzled me. I first noticed this } when showing people how to do specimen exchanges in TEM's in which a } premature turning of the specimen arm } before sufficient pumping on the airlock causes the high-voltage to shut } down. Sometimes it would take around 20 minutes to get the scope back on } line, and there can actually be introduction of a bit of oil into the } column. } } Needless to say, I wanted to warn trainees about this, so I first started } telling them something like "Insert the specimen arm, BUT DO NOT TURN IT } UNTIL....." Almost invariably, this resulted in exactly what I wanted to } avoid, usually the first or second } time I wasn't there to watch. Finally, I switched to saying "Insert the } specimen arm and push it into place with the flat of your hand, then after } the light goes out, turn it clockwise". That seems to work. } } The point is, I guess, that in training people about things that can } potentially damage equipment, I have found it best NOT to say "Don't ever } do this!" It works much better (for me) to say "Do it like this." and } demonstrate a way that minimizes the } chance of an accident. Later on, after the habit has been established, I } can explain the reasons without causing bad things to happen. } } Has anyone else experienced this? Is this Edgar Allen Poe's "Imp of the } Perverse" or just, gulp, me? } } Randy } } Randy Tindall } EM Specialist } Electron Microscopy Core Facility } W122 Veterinary Medicine } University of Missouri } Columbia, MO 65211 } Tel: (573) 882-8304 } Fax: (573) 884-5414 } Email: tindallr-at-missouri.edu } Web: http://www.biotech.missouri.edu/emc/ }
James S. Romanow The University of Connecticut Physiology and Neurobiology Department Electron Microscopy Facility Unit 2242 354 Mansfield Road Beach Hall, Room 129 Storrs, CT 06269-2242
} Hi all, } } I would appreciate some advice on low temperature embedding in the Leica EM } AFS freeze substitution unit using LR gold. Sorry, since I am a beginner } (concerning TEM) some of my questions might sound a little odd. } } My aim is to do immunogold labelling, mainly on cell walls, with sections } from Arabidopsis roots. The plan is to high pressure freeze Arabidopsis } roots, freeze substitute them, and embed them in LR gold at low temperature } (-25 degrees). } } At the moment I am running a few tests before I start the real experiment. } And I am having trouble with the LR gold embedding. } } This is what I tried so far: } I followed the protocol for "FS and low temperature embedding in } LEICA-capsules" from the AFS handbook (5.2, p.35). I was using LR gold + } 0.5% Benzil (w/v) as embedding medium. I started polymerisation at -25 } degrees with the UV lamp (Leica EM UV). After 24h the resin was not yet } solidified, only the bottom half of the capsules looked like it was solid. } } My questions: } Does anybody have experience with low temperature embedding using LR gold } in the Leica EM AFS? Any ideas how long UV-polymerisation might take? (24h } was the information I got from the supplier for the LR gold). Or is there an } easier way of getting my specimens embedded, preferably in the Leica EM } AFS? } } Thanks a lot for your help, } } Regina
Regina,
LR Gold won't polymerize completely if there is oxygen present. The AFS is supposed to exclude O2 by evaporating some of the LN2, but if there is a lot of air movement around the machine (i.e., lots of people walking by, or in front of an air vent) then it doesn't work so well. Make sure the inside glass is in place during UV exposure.
If the bottom of the capsule is hard, you can pour off the top liquid, cut off the goopy layer and use the hard bottom layer containing your specimen.
You should also make sure you are not introducing water (frost or condensation) during processing. That will also prevent polymerization. You may also retain some from the specimen if substitution is not complete.
Ask if you have more questions.
Good luck,
Kim
------- Kim Rensing Ph.D. Dept. of Botany, UBC 6270 University Blvd Vancouver, BC, Canada V6T 1Z4
My procedure is to get out a box of razor blades and a bigger box of Band-Aids. Then I demonstrate how to trim a block - bloodlessly. Then I do it again, and again. The third trapezoid always has a base that is between .5 and .75 mm. Then, I explain that I cut myself twice in the first week and never again.
By the time I have finished and watched the first 10 minutes, I know whether there is going to be a need for transfusions or not. If not, I walk away for 20 minutes before I come back and inspect their work. I always make a point to repair those attempts that are not 'up top snuff' and gush over those that are. Then I make the gushers help the hindered until everyone is on the same page.
One lab that way, usually the second, and sectioning always goes 50% better than if I neglected to bring the Band-Aids. The first lab is always spent cleaning the microscope.
Train 'em up good.
I had a sign on the outer back of the revolving darkroom door, which was exposed whenever anyone entered and revolved it to all of those who looked when they heard its noise. "Please don't enter the darkroom with the lights on." And, I never fixed it or moved it. Somehow, after the first week, no one ever left those light on either!
Hope you are well. I'm getting new scopes within next two months. New TEM (FEI Technai 12T) and new ESEM (FEI Quanta 400) w/EDS. These days such riches remind me of the poor man who won a Lincoln but had no money for gas. There I'll sit for weeks after my Technai 12T is up and running, daintily cutting grids from mesh with dull iris scissors. Then I'll have to go to three Mile Island for uranium salts and to West Philadelphia for lead tailings under old exterior window sills. And while I'm doing those collections, I'll take a few hits by random gammas and then get mugged. Microscopy is wonderful. Well, all won't be sad. I can analyze the skin on my finger tips for contamination of Pb and U for no cost and under only slight vacuum in my Quanta, and they won't dry out and I won't get beam-burned.
The pre-installation costs are mounting to around $25,000 for three 208V (1 x 60 and 2 x 20A) supplies, removal of 30 ft. of base cabinetry, capping plumbing of three sinks, running a dead 60A line for 15 ft, removing 1 fluorescent and 2 incandescent fixtures, and installing 50' of sound proofing to reduce acoustic noise (of my screams!). We thankfully have avoided the cost of jacking up our end of the building to determine the cause of any vibrations, because there were none.
Cheers,
Fred
Frederick C. Monson, PhD Center for Advanced Scientific Imaging Schmucker II Science Center c/o Geology/Astronomy West Chester University South Church Street and Rosedale Ave West Chester, Pennsylvania, USA, 19383 Phone: 610-738-0437 FAX: 610-738-0437 fmonson-at-wcupa.edu CASI URL: http://darwin.wcupa.edu/casi/ WCUPA URL: http://www.wcupa.edu/ Visitors URL: http://www.wcupa.edu/_visitors/
} ---------- } From: Leona Cohen-Gould } Sent: Wednesday, September 4, 2002 9:40 AM } To: Lois Anderson; microscopy-at-sparc5.microscopy.com } Subject: Re: trainee } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } } } } Has anyone ever trained an inexperienced EM tech and if so do you have } } any suggested tactics? } } *************** } I have taught and EM course a number of times and have trained } technicians who had no background. Slow and steady wins the race. I } have found that taking the time to explain WHY things are done, and } WHAT the aims of each procedure are is very helpful. You can just } make people memorize techniques, but without understanding they will } always be automatons and won't be able to deal with anything } unexpected. So, don't just give them a dehydration protocol, explain } why you need to extract the water, etc. Also, take it one step at a } time, don't try to teach the person everything, tissue to grid, in } one fell swoop. } } The good ting is that you can teach this person how to do things the } way you like, and they don't have any conflicting ideas. } } Good luck, } Lee } -- } Leona Cohen-Gould, M.S. } Sr. Staff Associate } Director, Electron Microscopy Core Facility } Manager, Optical Microscopy Core Facility } Joan & Sanford I. Weill Medical College } of Cornell University } voice (212)746-6146 } fax (212)746-8175 } }
I am isolating a rare monocyte population by FACS and trying to look at it by TEM. on the first go around i isolated 8500 cells and the pathologists were unable to get images of any cells becuase the pellet was too small to see.
Are there any techniques to allow the imaging of very small numbers of cells?
thanks, --- Seth L. Ness M.D., Ph.D Fellow in Human Genetics Department of Human Genetics Mount Sinai School of Medicine
At 11:35 AM 9/3/2002, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Flog them until they get with the program. However, this does not adhere to ISO-9000 principles. But, who knows, perhaps this could someday be included?
You are not in the ether alone. I believe what happens is that sometimes when an operator, or anyone for that matter, reads instructions, they anticipate the next step in the procedure and sometimes they are wrong. We have all done this in simple things like assembling toys or anything with mundane instructions that seem intuitive when they aren't necessarily and have several outcomes or degrees of freedom. I have been scolded on more occasions than I want to recall by my wife for "NOT READING THE INSTRUCTIONS ALL THE WAY FIRST!" Me being an engineer has yet to impress her in these matters. She mentioned nothing about neuro-lingusitic programming whilst yelling this at me. Needless to say I had to take the thing apart again.
Peter
-----Original Message----- } From: Jim Romanow [mailto:bsgphy3-at-uconnvm.uconn.edu] Sent: Wednesday, September 04, 2002 3:22 PM To: microscopy-at-sparc5.microscopy.com
Randy, This is called Neuro-Linguistic Programming (NLP) by some. http://www.nlptraining.com/index.asp
Disclaimer: The above link is for your information only.
} From: "Tindall, Randy D." {TindallR-at-missouri.edu} } To: {microscopy-at-sparc5.microscopy.com} } X-OriginalArrivalTime: 04 Sep 2002 17:43:49.0465 (UTC) } } } In training or help to train dozens of people over the years, I have run } across one phenomenon that has always puzzled me. I first noticed this } when showing people how to do specimen exchanges in TEM's in which a } premature turning of the specimen arm } before sufficient pumping on the airlock causes the high-voltage to shut } down. Sometimes it would take around 20 minutes to get the scope back on } line, and there can actually be introduction of a bit of oil into the } column. } } Needless to say, I wanted to warn trainees about this, so I first started } telling them something like "Insert the specimen arm, BUT DO NOT TURN IT } UNTIL....." Almost invariably, this resulted in exactly what I wanted to } avoid, usually the first or second } time I wasn't there to watch. Finally, I switched to saying "Insert the } specimen arm and push it into place with the flat of your hand, then after } the light goes out, turn it clockwise". That seems to work. } } The point is, I guess, that in training people about things that can } potentially damage equipment, I have found it best NOT to say "Don't ever } do this!" It works much better (for me) to say "Do it like this." and } demonstrate a way that minimizes the } chance of an accident. Later on, after the habit has been established, I } can explain the reasons without causing bad things to happen. } } Has anyone else experienced this? Is this Edgar Allen Poe's "Imp of the } Perverse" or just, gulp, me? } } Randy } } Randy Tindall } EM Specialist } Electron Microscopy Core Facility } W122 Veterinary Medicine } University of Missouri } Columbia, MO 65211 } Tel: (573) 882-8304 } Fax: (573) 884-5414 } Email: tindallr-at-missouri.edu } Web: http://www.biotech.missouri.edu/emc/ }
James S. Romanow The University of Connecticut Physiology and Neurobiology Department Electron Microscopy Facility Unit 2242 354 Mansfield Road Beach Hall, Room 129 Storrs, CT 06269-2242
} (FEI Technai 12T) and new ESEM (FEI Quanta 400) w/EDS. These days such } riches remind me of the poor man who won a Lincoln but had no money for gas. } There I'll sit for weeks after my Technai 12T is up and running, daintily } cutting grids from mesh with dull iris scissors. Then I'll have to go to } three Mile Island for uranium salts and to West Philadelphia for lead } tailings under old exterior window sills.
Luxury! We're so poor we have to shrink chicken wire in the washing machine to make grids! C.
} And while I'm doing those } collections, I'll take a few hits by random gammas and then get mugged. } Microscopy is wonderful. Well, all won't be sad. I can analyze the skin on } my finger tips for contamination of Pb and U for no cost and under only } slight vacuum in my Quanta, and they won't dry out and I won't get } beam-burned. } } The pre-installation costs are mounting to around $25,000 for three 208V (1 } x 60 and 2 x 20A) supplies, removal of 30 ft. of base cabinetry, capping } plumbing of three sinks, running a dead 60A line for 15 ft, removing 1 } fluorescent and 2 incandescent fixtures, and installing 50' of sound } proofing to reduce acoustic noise (of my screams!). We thankfully have } avoided the cost of jacking up our end of the building to determine the } cause of any vibrations, because there were none. } } Cheers, } } Fred } } Frederick C. Monson, PhD } Center for Advanced Scientific Imaging } Schmucker II Science Center } c/o Geology/Astronomy } West Chester University } South Church Street and Rosedale Ave } West Chester, Pennsylvania, USA, 19383 } Phone: 610-738-0437 } FAX: 610-738-0437 } fmonson-at-wcupa.edu } CASI URL: http://darwin.wcupa.edu/casi/ } WCUPA URL: http://www.wcupa.edu/ } Visitors URL: http://www.wcupa.edu/_visitors/ } } } } ---------- } } From: Leona Cohen-Gould } } Sent: Wednesday, September 4, 2002 9:40 AM } } To: Lois Anderson; microscopy-at-sparc5.microscopy.com } } Subject: Re: trainee } } } } -------------------------------------------------------------------- ---- } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } } -------------------------------------------------------------------- ---. } } } } } } } } } } Has anyone ever trained an inexperienced EM tech and if so do you have } } } any suggested tactics? } } } } *************** } } I have taught and EM course a number of times and have trained } } technicians who had no background. Slow and steady wins the race. I } } have found that taking the time to explain WHY things are done, and } } WHAT the aims of each procedure are is very helpful. You can just } } make people memorize techniques, but without understanding they will } } always be automatons and won't be able to deal with anything } } unexpected. So, don't just give them a dehydration protocol, explain } } why you need to extract the water, etc. Also, take it one step at a } } time, don't try to teach the person everything, tissue to grid, in } } one fell swoop. } } } } The good ting is that you can teach this person how to do things the } } way you like, and they don't have any conflicting ideas. } } } } Good luck, } } Lee } } -- } } Leona Cohen-Gould, M.S. } } Sr. Staff Associate } } Director, Electron Microscopy Core Facility } } Manager, Optical Microscopy Core Facility } } Joan & Sanford I. Weill Medical College } } of Cornell University } } voice (212)746-6146 } } fax (212)746-8175 } } } } }
First of all, Sorry if some of you receive this email more than once, I'm sending this to 3 mailinglists at the same time... I have a question about a fluorophore. I'm looking for a secondary fluorescent antibody that has a really long life-time. The purpose is to inject fixed cells (staining before fixation) into a mice so I can measure the number of fluorescent cells in an organ after 60 days. I was thinking about carboxyfluorescein, but does it really has a long fluorescent life-time and/or are there any better secundary antibodies? Thank you in advance,
Greetings With 8500 cells it sounds like the pathologists lost them while processing the tissue (fixation, dehydration and infiltration). One way to circumvent this is to "embed" the recovered cells in a pellet of albumin and crosslinking the albumin with glutaraldehyde. Basically, you gently centrifuge the cells of interest (after fixation and osmication) down (6-800xG) in an eppendorf and resuspend in a tiny volume of buffer (say 20uL). Then, at the same time, add 50uL of 5% BSA and 50uL of 2% glutaraldehyde. The glut fixes and cross links the BSA with the cells of interest embedded within. Kind of like a cocoon. This is then spun down and can then be transferred from the eppendorf, dehydrated and embedded in EPON. It turns the 8500 cells into a tissue chunk. The BSA serves as a "carrier" that impedes the steady loss of cells after each sequential step. I was taught this technique back in the late 80's by a very well respected microscopist by the name of Wille or Willy. Look for references from UIC back in the 80's. Oh, the BSA doesn't interfere with images because it is not osmicated. I plan on doing some EM on FACS samples later this fall. Let me know what you decide to do or if I can be of further assistance.
Mike
At 08:04 PM 9/4/2002 -0400, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
At 04:39 AM 9/5/2002, you wrote: } Hi XLrs, } } I frequently get "Unable to Allocate Memory" errors when trying to save } images from MCTRL. Restarting Windows (NT) is the only way I have } discovered will fix it. Anyone know what is going on? } -- } --- } Regards, Cameron.
This is highly suspicious of a defective app... not WinNT. Unlike Win98, WinNT 4 & 5 handles memory totally differently, and very well. If the app does a malloc() and does not release the memory allocated, it is hung up. WinNT cannot perform garbage collection. I would suggest reporting this to the vendor as an app bug.
on 9/4/02 8:44 AM, Peter Tomic at PTomic-at-anadigics.com wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } A few additional comments - be sure to run a standard first for the Si. Peak broadening would be expected at the lower Sr location (+ the Si), so if you have a decent program, the separation can usually be done. As the others mentioned, the higher energy lines will confirm the Sr - you did not mention in your note if quant was desired; it sounds as though it is not necessary. If just the presence of the Sr is of interest, use those heavier lines...as Peter suggests, make sure the operating voltage is no lower than 25KeV..You'll need roughly double the energies to get your signal on these. One other question..you say 'on' (the Si). Knowing the depth of the Sr is important, too.
on 9/4/02 8:44 AM, Peter Tomic at PTomic-at-anadigics.com wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } } Bill; } } It's true that Si & Sr overlap at ~ 1.8 KeV. The Sr major La1 line is at } 1.806 KeV and the Si Ka1 major line is at 1.739 KeV. However, Sr is a much } more complex atom and has a Ka1 major line at 14.164 KeV as Bill Giles } mentioned below. Sr should be easily discernable from Si. Of course you } will have to have an incident electron energy of about 1.5 to 2X of the Sr } Ka1 energy to see it. I assume you can run your survey at 25 to 30 KeV? } } Peter Tomic } Anadigics, Inc. } } } } -----Original Message----- } } From: Giles, Bill [mailto:William.Giles-at-timet.com] } Sent: Tuesday, September 03, 2002 4:29 PM } To: 'Microscopy-at-MSA.Microscopy.Com' } Subject: RE: Strontium on Clinoptilolite } } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Try looking at 14.164 Kev, should be a K line down there. } } William Giles } Senior Electron Microscopist } Metallography Lab Coordinator } P.O. Box 2128 } Henderson, Nevada 89009 } (702) 566-4436 } (702) 564-9038 (Fax) } Bill.Giles-at-timet.com } } RE: } Hello all ! } Maybe somebody knows how to analyse samples of clinoptilolite containing } strontium on EDX detector. Strontium and Silicon have both peak in one line. } Please help me. This is my doc work. } } } } * } }
Over the years I have taught a score of students to use an ultramicrotome. I have evolved my approach so that I know start with a trimmed block that is mounted and ready to cut. Once they get sections, I back up the knife and start with the the simplest alignment along the y axis, then i move on to x-axis and finally z-axis alignment. when they get good at that, i switch to blocks that need progressively more trimming. I have learned that the final steps in microtomy are really the simplest if everything is perfect. When students understand where they are going, it is easier for them to learn the steps on how to get there. For example, it is hard for them to know how much to trim off or why a small block face is better if they have never seen a good block size or tried to thin section one that is too big.
-- Thomas E. Phillips, Ph.D. Associate Professor of Biological Sciences Director, Molecular Cytology Core Facility
3 Tucker Hall Division of Biological Sciences University of Missouri Columbia, MO 65211-7400 (573)-882-4712 (voice) (573)-882-0123 (fax)
Seth, I have sectioned cell fractions by putting the sample into a clean polypropylene eppendorf tube, centrifuge it well and do the total fixation -} embedding without disturbing the "pellet". Care must be taken to totally exchange the solutions. Repeat a step if there is a question. After the resin (epon) is hard the next morning, pop it out of the tube (I usually fill 1/4 of the tube with the final resin). The pellet should be visible on the side of the cone at the bottom - try using a dissecting microscope with the light under the the block. It is usually necessary to cut the cone to a flat side and glue it onto a blank so that it can be sectioned. Pat
Patricia Stranen Connelly The University of Pennsylvania Department of Biology Philadelphia, PA 91904-6018
Seth- This is a small number for EM preparation. If I were you, I would attach them to the bottom of one well in a 48-well plate using poly-lysine to afix them. Then, you could embed them by making a cast of the dish in epoxy resin. You need somebody reasonably adept in the lab to do this, but it isn't hard. Carol Heckman (Bowling Green State University)
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I'm working with a Sirion XL30 with Edax. MCTRL is running under WinNT4 and is integrated with Soft Imaging analySIS. Host computer is a Umax server. Never had a crash or memory problem or had to reboot.
I still think it is a MCTRL version problem. And, any system running Win 3.1 is an antique. If it is under contract, I would have expected FEI to upgrade the system (they would have to provide a new computer box to do this effectively since WinNT is set up for the PCI cards. The 3.1 system is most certainly ISA cards.) They probably don't want to put out the cost of upgrading.
I upgraded my Amray SEM control from Win 3.1 to Win95 and then to Win98SE. I used an ASUS motherboard with Pentium II 450MHz, 384MB RAM, dual 40G drives, Zip, floppy and SCSI Jaz drive. The motherboard has one ISA slot which I needed for the Nibblenet interface card. All of the other cards are PCI. The Robinson BSE control program works fine on any of the Win OS versions. Fortunately, it communicates via serial port.
gary g.
At 11:48 AM 9/5/2002, you wrote: } I had the same problem with my XL. FEI gave me no answers. I believe it } has something to do with the EDAX integration. I got the error after heavy } use of the EDAX software. } } Jon } } Gary Gaugler wrote: } } } ------------------------------------------------------------------------ } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } } -----------------------------------------------------------------------. } } } } At 04:39 AM 9/5/2002, you wrote: } } } Hi XLrs, } } } } } } I frequently get "Unable to Allocate Memory" errors when trying to save } } } images from MCTRL. Restarting Windows (NT) is the only way I have } } } discovered will fix it. Anyone know what is going on? } } } -- } } } --- } } } Regards, Cameron. } } } } This is highly suspicious of a defective app... not WinNT. Unlike } } Win98, WinNT 4 & 5 handles memory totally differently, and very } } well. If the app does a malloc() and does not release the memory } } allocated, it is hung up. WinNT cannot perform garbage collection. } } I would suggest reporting this to the vendor as an app bug. } } } } gary g.
having had to visualize pellet sizes of below 1000 peripheral blood monocytes in one earlier study of chlymidial infection, i can only say that i had mixed success in looking for essentially non-visable pellets. it may be a bit harsh to suggest that the pathologists simply lost the cells during processing. even after embedding in either agarose or albumin, the pellets, or embedded cores, will probably be only marginally visable, at best.
What is the computer system configuration? CPU, speed, physical memory, motherboard, disk, etc?
gg
At 03:03 PM 9/5/2002, you wrote: } Thought it might be appropriate to share our experience with the Memory } Allocation Error............ } } Our XL-40 was installed 3/97 as a stand alone 3.11 system. In 4/98 we } completed conversion to NT 4.0 then in 9/98 embedded our EDS system. Very } shortly thereafter (1 week), we began getting the dreaded Memory } Allocation Error. The error occured with varying frequency, ranging from } twice a day to twice a month. We found that a full PC shut down was } required to clear the error. Over the years we tried many things to get } rid of this error; to no avial. Following is a list of things we tried } which did NOT appear to affect the frequency of the error: } } 1. save images directly to the C drive } 2. save images directly to a network drive } 3. added more memory } 4. upgraded to XL v. 5.7 } 5. upgraded to service pack 4.0 } 6. changed out the PC (new Acer 11000) } 7. changed out the hard drive } 8. upgraded to service pack 5.0 } 9. upgraded to service pack 6a } 10. installed multi user login shell (account log) } } We found experimentally that the error could be induced by alternately } saving images and EDS spectra (about 20 each would usually do it). In } early May of this year, we acquired a new EDS-WDS system, which was } installed stand-alone (not embedded). We have not had a Memory Allocation } Error since! } } For what it's worth.................... } } Karen Dye } } } } } } begg.4-at-osu.edu 09/05/02 04:39AM } } } } Hi XLrs, } } I frequently get "Unable to Allocate Memory" errors when trying to } save images from MCTRL. Restarting Windows (NT) is the only way I } have discovered will fix it. Anyone know what is going on? } -- } --- } Regards, Cameron.
} } Hi there guys, } } } } I have a Tracor Northern MicroZ-II XEDS detector sat in my lab that I } } thought I might once be able to use. It has been kept cold since I } } inherited it about 6 years ago and I finally have to admit that I am never } } going to use it. So the question is, does anyone want it? It is a model } } D-1830 with the serial number 02880935. It has a microscope flange attached } } to it but I am unsure of the instrument that it came from. } } "Buyer" collects or pays shipping and no whining about it not working, it is } } as is. I haven't ever used it and so I have no idea if it works. The guy } } who gave it to me assured me that it worked when it came off his SEM but as } } I say that was 6 years ago. } } } } Any interest? Otherwise it goes to UM Property Disposition! } } } } } } -- } } John Mansfield PhD MInstP } } North Campus Electron Microbeam Analysis Laboratory } } 417 SRB, University of Michigan } } 2455 Hayward, Ann Arbor MI 48109-2143 } } Phone: (734) 936-3352 FAX (734) 763-2282 Cell. Phone: (734) 834-3913 } } (Leaving a phone message at 936-3352 is preferable to 834-3913) } } Email: jfmjfm-at-engin.umich.edu } } URL: http://emalwww.engin.umich.edu/people/jfmjfm/jfmjfm.html } } Location: Lat. 42! 16' 48" Long. 83! 43' 48" } }
you computer is over 5 years old, it's time to upgrade, by that i maean a whole new computer. with prices the way they are today for pcs it should be painless.
That is all very well, but when you computer runs a microscope that is under service contract and it is a microscope that is in use 20 hours per day, then upgrading it is not just a question of going to Best Buy and getting the latest e-Machines piece of you know what. FEI will not specify that their system will run with the latest computers and you also need one with an ISA slot and one that supports the video card they use to work with the overlay card that exists in the ISA slot. (I am talking legacy equipment here, the newer FEI systems use all PCI and have different configurations). Most of you know that having a service contract on the instrument permits you to have a gun change (a ten or so thousand dollar fix), if you have a tip go bad in a field emission instrument (your $26,000 a year service contract covers that). But it does not cover replacing the computer when it becomes so slow in comparison with the other systems in the lab that you think you are working on a Sinclair Spectrum!
On 9/6/02 8:48 AM, ""JHoffpa464-at-aol.com"-at-sparc5.microscopy.com" {"JHoffpa464-at-aol.com"-at-sparc5.microscopy.com} wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } you computer is over 5 years old, it's time to upgrade, by that i maean a } whole new computer. with prices the way they are today for pcs it should be } painless. } }
-- John Mansfield PhD MInstP North Campus Electron Microbeam Analysis Laboratory 417 SRB, University of Michigan 2455 Hayward, Ann Arbor MI 48109-2143 Phone: (734) 936-3352 FAX (734) 763-2282 Cell. Phone: (734) 834-3913 (Leaving a phone message at 936-3352 is preferable to 834-3913) Email: jfmjfm-at-engin.umich.edu URL: http://emalwww.engin.umich.edu/people/jfmjfm/jfmjfm.html Location: Lat. 42! 16' 48" Long. 83! 43' 48"
I hope you all understand that Microsoft isn't exactly telling the truth when it pops up a memory allocation error. Okay, maybe it is telling the truth, but the question is what truth?
Memory errors can pop up due to insufficient RAM on the computer (the kind you can add more of), insufficient GDI or USER space (more about that later), or even insufficient disk space (usually not a problem and easy to correct). I have seen all three labeled as "memory" errors and usually without a lot of hint as to which kind it was. The first and third issues are fairly easy to verify. The second can be more of a challenge.
For the first, you can hit Ctrl-Alt-Delete under Windows NT or 2000 and bring up the Task Manager to see how much memory is actually in use and how much remains free. Windows 9x (and 3.x, I think) have a utility program called SYSMON that can be installed to provide the same information. Both types of Windows provide a swap file on disk to virtually extend your memory beyond what can be held in the actual chips. It is slower to use the swap file than real memory, but it should allow your system to keep running even when it is allocating far more memory than is provided by the chips.
For the third, you should be able to open up a Windows Explorer window and see how much free space you have left on your disk(s). Admittedly, this is not the usual meaning of a memory error. (Disks are cheap now so there is USUALLY an abundance of space. However, older Windows 3 machines might be cramped for space.) However, I ran into one obscure program that needed workspace on a hard drive and the drive that workspace was on was filling up. The program itself, rather than Windows, coughed up the insufficient memory problem. But Windows could generate such an error if disk space is running low and Windows would like to extend the swap file but can't due to a lack of space.
The second issue could be more troublesome to track down but even more of a limitation. Windows allocates a small amount of memory, 64 kilobytes (not megabytes), to various bookkeeping tasks. Under Windows 3, a total of 64 kB was split between GDI (graphics stuff) and User (other various uses) stacks. Microsoft realized that wasn't enough so they gave each their own 64 kB chunk under Windows 9.x - but that can still be rather stingy. They also provided a tool, RSRCMTR.EXE, to track the use of that memory. (Rsrcmtr SEEMS to show a third type of resource, System, but that is really only the smaller of GDI and User.) Note that this small amount of memory is set aside by Windows and it doesn't matter if your machine is loaded with 512 MB of SDRAM. You only get 64 KB each for GDI and User memory!! (I would like to say something about Windows NT here, but I have recently made the transition and cannot authoritatively say how they handle the issue. It might be better.)
BTW, when GDI and/or User resources are depleted, any number of strange symptoms can appear: icons can lose their appearance, icon names can disappear or get corrupted, dialog boxes can turn illegible, etc. Basically, you will notice.
As programs are loaded, GDI and User and regular memory will get consumed. Some ill-written programs can allocate any or all of these three types of memory and forget to free them up when they are done with them. This can happen as the program runs continuously and documents are opened and closed, or as the program is repeatedly started and stopped and restarted. I have encountered many such programs over the years - even earlier versions of Excel and Eudora were notorious for such behavior (chewing up GDI and/or User memory). If it is a problem, it falls to the author to root out the bug and fix it, and most authors do just that.
All that said, I don't know which flavor of memory problem you have. Hopefully, you can determine that for yourself from my comments above and pin down the problem. If you have further questions, feel free to ask.
Now I would like to hear from any NT gurus out there - what are the rules for GDI and User space under NT and is there a good utility for tracking their level? I have recently jumped to Windows 2000 and could find myself facing the same issues as the original poster.
Warren
At 04:17 PM 9/5/02 -0700, you wrote:
} What is the computer system configuration? CPU, speed, } physical memory, motherboard, disk, etc? } } gg } } At 03:03 PM 9/5/2002, you wrote: } } Thought it might be appropriate to share our experience with the Memory } } Allocation Error............ } } } } Our XL-40 was installed 3/97 as a stand alone 3.11 system. In 4/98 we } } completed conversion to NT 4.0 then in 9/98 embedded our EDS } } system. Very shortly thereafter (1 week), we began getting the dreaded } } Memory Allocation Error. The error occured with varying frequency, } } ranging from twice a day to twice a month. We found that a full PC shut } } down was required to clear the error. Over the years we tried many } } things to get rid of this error; to no avial. Following is a list of } } things we tried which did NOT appear to affect the frequency of the error: } } } } 1. save images directly to the C drive } } 2. save images directly to a network drive } } 3. added more memory } } 4. upgraded to XL v. 5.7 } } 5. upgraded to service pack 4.0 } } 6. changed out the PC (new Acer 11000) } } 7. changed out the hard drive } } 8. upgraded to service pack 5.0 } } 9. upgraded to service pack 6a } } 10. installed multi user login shell (account log) } } } } We found experimentally that the error could be induced by alternately } } saving images and EDS spectra (about 20 each would usually do it). In } } early May of this year, we acquired a new EDS-WDS system, which was } } installed stand-alone (not embedded). We have not had a Memory } } Allocation Error since! } } } } For what it's worth.................... } } } } Karen Dye } } } } } } } } } begg.4-at-osu.edu 09/05/02 04:39AM } } } } } Hi XLrs, } } } } I frequently get "Unable to Allocate Memory" errors when trying to } } save images from MCTRL. Restarting Windows (NT) is the only way I } } have discovered will fix it. Anyone know what is going on? } } } } Regards, Cameron.
------------------------------------------- No files should be attached to this message ------------------------------------------- Warren E. Straszheim, Ph.D. Materials Analysis and Research Lab Iowa State University 23 Town Engineering Ames IA, 50011-3232
I hope to hear from anyone with good or bad personal experience with lasik or other corrective eye surgery. I am particularly anxious to know if the surgery adversely affected vision through microscope binoculars, and the difficulties with loosing near vision (I take my glasses off for close work).
Many thanks,
Doug
---------------------- Douglas R. Keene Micro-Imaging Center Shriners Hospital for Children 3101 S.W. Sam Jackson Park Road Portland, Oregon 97239 Phone: 503-221-3434 FAX: 503-412-6894
I always used to start by teaching them how to make glass knives. This conveys the idea that we're dealing with very small things that need enormous attention to detail. From there, I used to show them how to process tissue, then how to trim a block and then move on to thick sections, thin sections, staining, and finally using the microscope. The continuity of following their own work from beginning to end made it more interesting, and therefore memorable, for them. I also took care to explain why we needed to do each individual action, and what would happen if we didn't. I gave each one a copy of my lab manual, but I also insisted that they add their own thoughts as we proceeded. All this is in the past tense because I took early retirement as soon as I could. This, along with endless patience and a sense of humour, is also necessary.
Well said, John. This is an issue that has been creeping up on us since microscopes became intimately attached to computers. My 1983 Philips 410LS runs pretty well with no RS232 and a stand-alone Gatan CCD. But my 1998 Hitachi SEM is a bit slow since it is tied to Windows 95. Hitachi informs me that an upgrade to Windows NT 4.0 (that's right; not even Windows 2002 or XP) will cost close to $20K. We benefit from the versatility of a computer interface but the manufacturer benefits from selling machines that have the life span of a computer.
Rick A. Harris, Director Microscopy and Imaging Facility Section of Molecular and Cellular Biology 1241 Life Sciences Addition University of California Davis, CA 530 752 2914 http://katie.ucdavis.edu raharris-at-ucdavis.edu
At 11:36 AM 9/6/2002 -0400, John F. Mansfield wrote: } ----------------------------------------------------------. } } } That is all very well, but when you computer runs a microscope that is under } service contract and it is a microscope that is in use 20 hours per day, } then upgrading it is not just a question of going to Best Buy and getting } the latest e-Machines piece of you know what. FEI will not specify that } their system will run with the latest computers and you also need one with } an ISA slot and one that supports the video card they use to work with the } overlay card that exists in the ISA slot. (I am talking legacy equipment } here, the newer FEI systems use all PCI and have different configurations). } Most of you know that having a service contract on the instrument permits } you to have a gun change (a ten or so thousand dollar fix), if you have a } tip go bad in a field emission instrument (your $26,000 a year service } contract covers that). But it does not cover replacing the computer when it } becomes so slow in comparison with the other systems in the lab that you } think you are working on a Sinclair Spectrum! } } On 9/6/02 8:48 AM, ""JHoffpa464-at-aol.com"-at-sparc5.microscopy.com" } {"JHoffpa464-at-aol.com"-at-sparc5.microscopy.com} wrote: } } } ------------------------------------------------------------------------ } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } } -----------------------------------------------------------------------. } } } } } } you computer is over 5 years old, it's time to upgrade, by that i maean a } } whole new computer. with prices the way they are today for pcs it should be } } painless. } } } } } } -- } John Mansfield PhD MInstP } North Campus Electron Microbeam Analysis Laboratory } 417 SRB, University of Michigan } 2455 Hayward, Ann Arbor MI 48109-2143 } Phone: (734) 936-3352 FAX (734) 763-2282 Cell. Phone: (734) 834-3913 } (Leaving a phone message at 936-3352 is preferable to 834-3913) } Email: jfmjfm-at-engin.umich.edu } URL: http://emalwww.engin.umich.edu/people/jfmjfm/jfmjfm.html } Location: Lat. 42! 16' 48" Long. 83! 43' 48"
} Now I would like to hear from any NT gurus out there - what are the rules } for GDI and User space under NT and is there a good utility for tracking } their level? I have recently jumped to Windows 2000 and could find myself } facing the same issues as the original poster.
Any good programmer should be able to identify a leaking program. Tracking the leak back to the source code can be time consuming but is not impossible. Checking for memory leaks is (or should be) part of any software program testing procedure.
I had Lasix in February with spectacular results, it was worth every penny I spent. I have 20/20 distance vision now plus good vision up close (8 inch WD) for fine work. I have some slight "Starburst" refraction at night but it is does not effect my night vision. I am active in Astronomy too with a large telescope at my disposal and notice no detrimental effects from the surgery. As for the work at the Microscope or Microtome I think it is much better than before I have the corrective surgery.
The most important thing is to choose a Lasix center that does the procedure under "real" operating room conditions vs clean room environments like some of the "Vi son Mills" in Malls have. I took my time and shopped around not for the best price but the best center & surgeon.
--- Albert Coritz --- cactusgrower-at-earthlink.net Sales Manager EMS/ Diatome USA
} [Original Message] } From: Doug Keene {drk-at-shcc.org} } To: {Microscopy-at-sparc5.microscopy.com} } Date: 9/6/2002 11:37:44 AM } Subject: corrective eye surgery } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Hello Microscopists, } } I hope to hear from anyone with good or bad personal } experience with lasik or other corrective eye surgery. I } am particularly anxious to know if the surgery adversely } affected vision through microscope binoculars, and the } difficulties with loosing near vision (I take my glasses } off for close work). } } Many thanks, } } Doug } } ---------------------- } Douglas R. Keene } Micro-Imaging Center } Shriners Hospital for Children } 3101 S.W. Sam Jackson Park Road } Portland, Oregon 97239 } Phone: 503-221-3434 } FAX: 503-412-6894 }
Scott, That's fine if you are the software developer. I am a little old academic using programs like MS word, netscape, photohop, acrobat reader, and a few others on my computer. Nothing too wild. Well these programs definitely leak memory. Once in a while I must restart the computer after getting bogus memory errors. I suspect the Microsoft products. But I havn't found any way for an ordinary user such as myself to figure out *which* program is actually leaking.
Tobias
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I would be interested in hearing from anyone who has put a photographic strobe into a microscope stand, on the cheap, for better photos. Reflected light on Stereomicroscope is obvious; I am thinking of kohler illumination. My limited experiments, wven with a digital camera, have revealed exposure times to be limiting, not to mention vibration.
Alan Davis Marianas High School, Saipan
-- adavis-at-saipan.com 1-670-322-6580 Alan E. Davis, PMB 30, Box 10006, Saipan, MP 96950-8906, CNMI
I have steadily endeavored to keep my mind free, so as to give up any hypothesis, however much beloved -- and I cannot resist forming one on every subject -- as soon as facts are shown to be opposed to it. -- Charles Darwin (1809-1882)
The right to search for truth implies also a duty; one must not conceal any part of what one has recognized to be true. -- Albert Einstein
As we enjoy great advantages from the inventions of others we should be glad of an opportunity to serve others by any invention of ours, and this we should do freely and generously. -- Benjamin Franklin
The problem of software compatibility between machines and operating system versions is one which plagues not only users, but also manufacturers.
I began my career in this industry writing assembly code for the "minicomputers" that were just starting to be tied to pulse-height analyzers in the early 1970s. The challenge, of course, was to perform useful work in a 4K environment where not even disk storage was available (and yes, I mean 4K, not 4M or 4G). When we added peripherals, we had to write our own drivers -- and even mathematical algorithms needed to be coded from scratch since computations generally had to be done in "fixed point". The upside was that a programmer knew EXACTLY what was in the computer and, after sufficient testing, could feel pretty confident about how the code would perform under all plausible circumstances. Sure, we still introduced our "bugs" -- and I introduced my share (as some members of this listserver can personally testify) -- but we could figure them out by duplicating the circumstances back in the factory. In extreme cases, you could take your debugging right down to the individual machine instruction -- and frequently did.
Life has changed. Today, I'm sure that there is not a single human who fully understands all of the intricacies of the Windows operating system (and some days I think mankind in aggregate is clueless) -- not to mention all of the complexities that occur with the addition of peripherals, utility software, and software development tools such as compilers, linkers, library functions etc. -- look at a typical desktop PC and there are probably thousands of people who have had a role in establishing the integrity of the code that it is running. Sure, modern operating systems impose barriers and structures such that programs run independently, at least in principle, and IN PRINCIPLE, it should be possible to freely switch between computers and add peripherals and capabilities without incurring any problems. Some day that may be possible -- but that day hasn't yet fully arrived.
The reality is that there remain many subtle ways in which programs can behave properly in one environment, and not in another. With appropriate care in programming practice, problems due to these things are rare, but when they do occur, they are extremely difficult to isolate -- and costly, especially when they need to be figured out in the customer's lab. Sometimes, the problem isn't even the fault of the application programmer -- anyone who does this stuff (or manages it) can tell you horror stories about undocumented bugs in compilers, operating systems, and device drivers. The programmer's challenge in many cases is figuring out how to get his/her stuff to run properly when the tools she/he must work with aren't doing what they're supposed to.
Back in the days when instruments were "hard wired", they simply went obsolete in a relatively short time (5 years wasn't unusual), and the user knew he/she had to purchase a new one to get the latest/greatest features. As we have moved into a "software" age, manufacturers have been able to provide software updates that add features and prolong the life of the hardware. But as software environments have grown more complicated and user expectations more demanding (and properly so), manufacturers' software development and support costs have also grown exponentially. Keep in mind that manufacturers of EM equipment don't enjoy the luxury of large sales volumes, and it is easy to see that hiring a battery of people to test software under every possible variant of computer, operating system, and peripheral configuration just isn't feasible. So the only real practical approach is to warrant system performance as it leaves the factory. Though most of us would love to be nice guys and say -- "sure, just upgrade to a new computer when you feel like it", users have a way of becoming testy and accusative when they can't get the instrument to work properly with the new hardware (at least I am when I find myself in this situation). One solution is to tell the user "upgrade at your own risk" -- but this tends to generate ill will. The only realistic alternative is for the manufacturer to take responsibility for the configuration -- and this is an expensive proposition.
So, though I appreciate and share the pain of having to buy expensive factory upgrades (remember, we manufacturers buy stuff from other vendors and have similar problems), I just want to point out that the presumption that the "manufacturer benefits from selling machines that have the life span of a computer" isn't the "gold mine" that it might appear to be (ah -- if only that were the case!)
Fred Schamber ASPEX LLC
Rick Harris wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } Well said, John. This is an issue that has been creeping up on us since } microscopes became intimately attached to computers. My 1983 Philips 410LS } runs pretty well with no RS232 and a stand-alone Gatan CCD. But my 1998 } Hitachi SEM is a bit slow since it is tied to Windows 95. Hitachi informs } me that an upgrade to Windows NT 4.0 (that's right; not even Windows 2002 } or XP) will cost close to $20K. We benefit from the versatility of a } computer interface but the manufacturer benefits from selling machines that } have the life span of a computer. } } Rick A. Harris, Director } Microscopy and Imaging Facility } Section of Molecular and Cellular Biology } 1241 Life Sciences Addition } University of California } Davis, CA } 530 752 2914 } http://katie.ucdavis.edu } raharris-at-ucdavis.edu } } At 11:36 AM 9/6/2002 -0400, John F. Mansfield wrote: } } ----------------------------------------------------------. } } } } } } That is all very well, but when you computer runs a microscope that is under } } service contract and it is a microscope that is in use 20 hours per day, } } then upgrading it is not just a question of going to Best Buy and getting } } the latest e-Machines piece of you know what. FEI will not specify that } } their system will run with the latest computers and you also need one with } } an ISA slot and one that supports the video card they use to work with the } } overlay card that exists in the ISA slot. (I am talking legacy equipment } } here, the newer FEI systems use all PCI and have different configurations). } } Most of you know that having a service contract on the instrument permits } } you to have a gun change (a ten or so thousand dollar fix), if you have a } } tip go bad in a field emission instrument (your $26,000 a year service } } contract covers that). But it does not cover replacing the computer when it } } becomes so slow in comparison with the other systems in the lab that you } } think you are working on a Sinclair Spectrum! } } } } On 9/6/02 8:48 AM, ""JHoffpa464-at-aol.com"-at-sparc5.microscopy.com" } } {"JHoffpa464-at-aol.com"-at-sparc5.microscopy.com} wrote: } } } } } ------------------------------------------------------------------------ } } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } } } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } } } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } } } -----------------------------------------------------------------------. } } } } } } } } } you computer is over 5 years old, it's time to upgrade, by that i maean a } } } whole new computer. with prices the way they are today for pcs it should be } } } painless. } } } } } } } } } } -- } } John Mansfield PhD MInstP } } North Campus Electron Microbeam Analysis Laboratory } } 417 SRB, University of Michigan } } 2455 Hayward, Ann Arbor MI 48109-2143 } } Phone: (734) 936-3352 FAX (734) 763-2282 Cell. Phone: (734) 834-3913 } } (Leaving a phone message at 936-3352 is preferable to 834-3913) } } Email: jfmjfm-at-engin.umich.edu } } URL: http://emalwww.engin.umich.edu/people/jfmjfm/jfmjfm.html } } Location: Lat. 42! 16' 48" Long. 83! 43' 48"
on 9/4/02 1:43 PM, Tindall, Randy D. at TindallR-at-missouri.edu wrote:
} In training or help to train dozens of people over the years, I have run } across one phenomenon that has always puzzled me. I first noticed this when } showing people how to do specimen exchanges in TEM's in which a premature } turning of the specimen arm before sufficient pumping on the airlock causes } the high-voltage to shut down. Sometimes it would take around 20 minutes to } get the scope back on line, and there can actually be introduction of a bit of } oil into the column. } } Needless to say, I wanted to warn trainees about this, so I first started } telling them something like "Insert the specimen arm, BUT DO NOT TURN IT } UNTIL....." Almost invariably, this resulted in exactly what I wanted to } avoid, usually the first or second time I wasn't there to watch. Finally, I } switched to saying "Insert the specimen arm and push it into place with the } flat of your hand, then after the light goes out, turn it clockwise". That } seems to work. } } The point is, I guess, that in training people about things that can } potentially damage equipment, I have found it best NOT to say "Don't ever do } this!" It works much better (for me) to say "Do it like this." and } demonstrate a way that minimizes the chance of an accident. Later on, after } the habit has been established, I can explain the reasons without causing bad } things to happen. } } Has anyone else experienced this? Is this Edgar Allen Poe's "Imp of the } Perverse" or just, gulp, me? } Dear Randy, Sue and I have a saying that the universe doesn't hear "not". I would say, "Insert the specimen arm, then stop." I could then explain that one has to wait for the vacuum to be established, etc. (In microscopes with a vacuum-ready indicator, you could say, "...stop until the light goes on.") On a humid day, you could explain that the electrons need a vacuum on the inside of the column, and the trainee needs the air on the outside, so the pumpdown is necessary to go from outside to inside, during the time you are waiting to introduce the next step. Yours, Bill Tivol
We have a shutter that has become sticky opening and closing. Does anyone have any suggestions concerning an appropriate lubricant to apply to the leaves to try and smooth its motion. Thanks- Dave
Oils should not be used to lubricate leaf shutters or iris diaphragms. Paradoxically, instead of acting as a lubricant the surface tension of the oil film will bind the leaves together and prevent them from sliding freely. Problems with sticking are likely caused by dust or a particle of grit, a buildup of crud somewhere, excessive wear or mechanical damage. Careful cleaning of the shutter may be a better bet. Chris
----- Original Message ----- } From: "David Knecht" {knecht-at-uconn.edu} To: "microscopy" {microscopy-at-sparc5.microscopy.com} Sent: Sunday, September 08, 2002 5:51 PM
If it is a Vincent Assoc. Uniblitz shutter, don;t apply anything to it. Call them.
On Sun, 8 Sep 2002, David Knecht wrote: } We have a shutter that has become sticky opening and closing. Does } anyone have any suggestions concerning an appropriate lubricant to } apply to the leaves to try and smooth its motion. Thanks- Dave } } }
Contact Miller-Stephenson Chemical Company at (203)743-4447 or (818)896-4714. Ask for the MS-143V or MS-145 for brush, not the aerosol. They provide free samples. You may specify the amount of dry lubricant in the fluid. 1% to 5% is all you need.
Both these products are used as dry lubricants and mold release agents. Both are solids suspended in volatile fluid. High vacuum compatible. I use those on JEOL TEMs mechanical shutter blades (pretty large blades) under the viewing screen, as well as on other mechanisms.
Make sure that the shutter blades are squeaky clean, before applying these products. No dust, oil, fibers, etc.
Vitaly Feingold Scientific Instruments and Applications 2773 Heath Lane, Duluth GA 30096 (770)232-7785 ph. (770)232-1791 fax (678)467-0012 mobile
This message is made of 100% recycled electrons. ----- Original Message ----- } From: David Knecht {knecht-at-uconn.edu} To: microscopy {microscopy-at-sparc5.microscopy.com} Sent: Sunday, September 08, 2002 12:51 PM
Does anyone have a method to de-plasticize sections in Spurr resin that can allow immunohist to be done on them? Thanks. Stacey Andringa
My name is Terry Ellis I work for Hallmark Cards Inc. and I run their SEM-EDX equipment and also use a metallurgical, stereo and regular microscope for sample prep and various projects. I am a diabetic and have had several eye problems and surgeries. one, the Doctor used a laser several to tack down my retina this has reduced my night vision some but hasn't affected my microscope use. Two, I had a detached retina in one eye then a year later a blood vessel burst in the other eye, both times the doctor used microsurgery to remove the fluid in my eye and lasers to correct the problems. Thank goodness I still can see fine with both eyes, I have had to use a hat and dark glasses since the body fluid that replaced the old fluid gel is much clearer and I am more sensitive to light, on the microscopes I just use less light. Three, I had to have the lenses in both eyes replaced due to cataracts in them, one lenses for distance and the other lens for close-up, I have set up the binocular microscopes for my eyes by setting one eye piece in focus then setting the other eye piece, which has an separate focus knob, in focus then I can use the microscopes focus knobs to bring it all in focus, which means that no one else can use them but I have a camera and monitor that I move and set up for each microscope when some one else needs to see what I see. Four, I developed glaucoma in one eye and another Doctor put in what he called a valve in it to relieve the pressure. I have lost some vision in that eye but have been able to adjust the binoculars so I can almost see as good with the bad eye but I generally use just one eye since I tend to get headaches when I use both a lot. During the surgery's I could only see with one eye and my boss still calls me the one eyed microscopist. Terry Ellis tellis2-at-hallmark.com 816-545-6573
Stacey: The deplasticization techniques using sodium methoxide (do a quick search at Pubmed, or check some of the classic biological TEM books for the exact recipes) is the only way I know to remove any of the epoxies from samples. Whether or not you are going to have any antigen expression left can only be determined by doing the experiment.
Roger Moretz, Ph.D. Dept of Toxicology Boehringer Ingelheim Pharmaceuticals Ridgefield, CT -- Where the world is only slightly less weird than it actually is. } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Does anyone have a method to de-plasticize sections in Spurr resin that } can allow immunohist to be done on them? } Thanks. } Stacey Andringa } }
I have started taping myself with a digital video camera running through a procedure such as critical point drying or preparing formvar coated grids. I transfer this session to my Mac and use iMovie to edit the session, then burn it to a CD-ROM. My students are given this custom-made CD before meeting me in the lab. Since they have now seen the procedure demonstrated in my lab using my protocols, I quiz them on the details of the procedure, then dismiss those who fail the quiz and have them return at a later date to quiz again. Those who pass are then required to demonstrate the procedure. I can then give them individualized help on anything they have a problem with during the procedure. Upon successfully and safely completing the procedure, the user is considered 'checked out' on the procedure and able to use that procedure or equipment unsupervised.
The CD enables users to review a given procedure. It is often difficult for new trainees to make detailed enough notes that capture all the nuances. With the CD, however, they can easily back up and review complex sections. If they have been off cloning for the last 4 months and forgotten all the steps of a procedure, they have the CD-ROM to review.
This approach has cut down on my demo-as-training time and is changing how I teach my TEM protocols lab. The time I used to spend doing demo-training is shifting more toward protocol check-out. My first attempts using these customized CD-ROMS were enthusiastically encouraged by my SEM students last semester.
Steve
-- Dr. Steven Barlow EM Facility/Biology Dept. San Diego State University 5500 Campanile Drive San Diego CA 92182-4614 phone: (619) 594-4523 fax: (619) 594-5676 email: sbarlow-at-sunstroke.sdsu.edu http://www.sci.sdsu.edu/emfacility
Chairman, Educational Outreach subcommittee promoting microscopy instruction and increased access to microscopes Microscopy Society of America http://www.msa.microscopy.com/
I hope this is not some notion of a joke. It's a bad subject to joke about. This all sounds highly improbable. I doubt whether Ray Charles would have this many issues with vision.
PT
-----Original Message----- } From: Terry E Ellis [mailto:tellis2-at-hallmark.com] Sent: Monday, September 09, 2002 9:19 AM To: microscopy-at-sparc5.microscopy.com
My name is Terry Ellis I work for Hallmark Cards Inc. and I run their SEM-EDX equipment and also use a metallurgical, stereo and regular microscope for sample prep and various projects. I am a diabetic and have had several eye problems and surgeries. one, the Doctor used a laser several to tack down my retina this has reduced my night vision some but hasn't affected my microscope use. Two, I had a detached retina in one eye then a year later a blood vessel burst in the other eye, both times the doctor used microsurgery to remove the fluid in my eye and lasers to correct the problems. Thank goodness I still can see fine with both eyes, I have had to use a hat and dark glasses since the body fluid that replaced the old fluid gel is much clearer and I am more sensitive to light, on the microscopes I just use less light. Three, I had to have the lenses in both eyes replaced due to cataracts in them, one lenses for distance and the other lens for close-up, I have set up the binocular microscopes for my eyes by setting one eye piece in focus then setting the other eye piece, which has an separate focus knob, in focus then I can use the microscopes focus knobs to bring it all in focus, which means that no one else can use them but I have a camera and monitor that I move and set up for each microscope when some one else needs to see what I see. Four, I developed glaucoma in one eye and another Doctor put in what he called a valve in it to relieve the pressure. I have lost some vision in that eye but have been able to adjust the binoculars so I can almost see as good with the bad eye but I generally use just one eye since I tend to get headaches when I use both a lot. During the surgery's I could only see with one eye and my boss still calls me the one eyed microscopist. Terry Ellis tellis2-at-hallmark.com 816-545-6573
We are being asked for information about tables to put a microscope system on in a new lab being built. I wonder if anyone has suggestions on what to look for in a microscope table or specific brands if known. We are not planning an air table for this system. I should note that when Leica spec'd our new SP2 confocal, they claimed we did not need an air table, and so far they have been proven right. Hopefully the new building will be as stable. Right now, the microscope in question (Zeiss axio 200) is on a heavy duty generic metal table, on which we have placed a heavy stone benchtop slab supported by antivibration pads (audiophile variety). That has worked OK so far, but any suggestions given the chance to purchase something new are welcome. Thanks- Dave
here is what I am after. We have a self-made heating stage for an SEM, that can go up to 400°C. For thermal insulation the heater is mounted on a glass rod. When trying to mount everything I have broken the rod &-[.
Does anyone know where I can order glass or ceramics rods (or any oder material tha can take 400°C). Our former supplier is not available anymore. I need the following size: diameter 10 mm and lenght 120 mm. Is there a supplier in germany ?
Thanks for the help.
Andreas M.
Moritz Andreas Meyer Dipl.-Ing. (FH), MSc. Materials Analyst Materials Analysis Laboratory
AMD Saxony Limited Liability Company & Co. KG Wilschdorfer Landstraße 101 M/S E23-MA D-01109 Dresden F. R. Germany
We have an Olympus FV-300 confocal system for which we initially used tables a la carte. The arrangement took up much space and left parts of the system inaccessible. We have been forced to move the confocal system to a smaller room which cannot accommodate the three tables on which we had the system spread. Ten feet of space has dictated the table/rack configuration and selection. The table on which we are locating the microscope is sized to take the anti-vibration slab on which the microscope and detector/confocal box are located. Then a second table for the computer boxes and monitor and a third for the laser rack and power supplies. I worked directly with the primary supplier (NOT the company from which we are buying!) to insure that the design was consistent with our needs. The circuitous purchase route was required by the fact that the primary supplier expected payment on delivery (from an educational establishment?) whereas the microscope supplier knew better. My point is that for us the space to which we moved the system dictated the support system and its distribution. Finally, our three tables/racks ARE being custom made and were purchased ($2,000) through the company that supplied the confocal system itself. Something similar can be seen on the back page of the Fluoview brochure which can be downloaded as PDF from:
Beyond the issues enumerated, I agree, that nothing special is required. I ended up with hand-drawn plans for the pieces which I attached to the quote as specifications.
Regards,
Fred Monson
Frederick C. Monson, PhD Center for Advanced Scientific Imaging Schmucker II Science Center c/o Geology/Astronomy West Chester University South Church Street and Rosedale Ave West Chester, Pennsylvania, USA, 19383 Phone: 610-738-0437 FAX: 610-738-0437 fmonson-at-wcupa.edu CASI URL: http://darwin.wcupa.edu/casi/ WCUPA URL: http://www.wcupa.edu/ Visitors URL: http://www.wcupa.edu/_visitors/
THINKING IS MUCH MORE DIFFICULT THAN MEMORIZING.
} ---------- } From: David Knecht } Sent: Monday, September 9, 2002 11:10 PM } To: microscopy } Subject: Microscope table } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } We are being asked for information about tables to put a microscope } system on in a new lab being built. I wonder if anyone has suggestions } on what to look for in a microscope table or specific brands if known. } We are not planning an air table for this system. I should note that } when Leica spec'd our new SP2 confocal, they claimed we did not need an } air table, and so far they have been proven right. Hopefully the new } building will be as stable. Right now, the microscope in question } (Zeiss axio 200) is on a heavy duty generic metal table, on which we } have placed a heavy stone benchtop slab supported by antivibration pads } (audiophile variety). That has worked OK so far, but any suggestions } given the chance to purchase something new are welcome. Thanks- Dave } } }
Peter: No its all true, I wish it wasn't but it is true. I have been a type 1 Diabetic since 1963. Check out Diabetes and its long term complications. I didn't mention it but I have also been diagnosed with the start of renal kidney failure. I am on a vegetarian diet to slow down the failure rate and with a couple of pills it has slowed down. I also didn't mention a bad sprain that I did about 5 months ago that didn't heal and stayed swollen and the foot doctor said this has caused the calcium to be leached out of my foot so he has had me on crutches for the past two months until the foot heals and the bones in my foot recalcifly. I posted this in reply to a question about lasic surgery and meant to encourage the questioner to do what he needed to do. Really the fact that I work with microscopes has been a plus since I have been able to make up for my eye problems and still do my job to my bosses satisfaction. With a lot of other jobs I would have been out of work. No Joke Terry Ellis
David, We have several Vibraplane air tables (nitrogen) by Kinetic Systems which we are very happy with. Mike D.
David Knecht wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } We are being asked for information about tables to put a microscope } system on in a new lab being built. I wonder if anyone has suggestions } on what to look for in a microscope table or specific brands if known. } We are not planning an air table for this system. I should note that } when Leica spec'd our new SP2 confocal, they claimed we did not need an } air table, and so far they have been proven right. Hopefully the new } building will be as stable. Right now, the microscope in question } (Zeiss axio 200) is on a heavy duty generic metal table, on which we } have placed a heavy stone benchtop slab supported by antivibration pads } (audiophile variety). That has worked OK so far, but any suggestions } given the chance to purchase something new are welcome. Thanks- Dave
Hi all I would like to thank, on behalf of the ICEM15 committee, all those attended the ICEM 15 conference held in Durban, South Africa last week. We realised that getting people to come down South to South Africa would be a first for most, but we were overwhelmed with the numbers that did attend. It also caught the manufacturers, who hosted brilliant social functions, a little off guard too
We have started to change the website to accommodate the "after party pictures" and have copies of the programme etc available to you. Please let us know if we can assist in any way.
Again thanks to all who attended and see you all in Japan in 2006.
P.S. Nestor, do you think that the photo of you and me at the meet and greet function could be worth money?
} } } } I have only one functioning eye (since birth) and was asked by the } } researcher who wanted to hire me if it would be a problem running the } } scanning microscope. I told him I could watch TV for hours without a } } problem. The screen of the scope was not much different so I was and am a } } successful SEM operator. I can't evaluate stereo images or make use of a } } stereo microscope but I can still use them. } } } } Ron } } ----- Original Message ----- } } } From: "Terry E Ellis" {tellis2-at-hallmark.com} } } To: {microscopy-at-sparc5.microscopy.com} } } Sent: Tuesday, September 10, 2002 8:32 AM } } Subject: really no joke } } } } } } } ------------------------------------------------------------------------ } } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } } } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } } } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } } } -----------------------------------------------------------------------. } } } } } } } } } Peter: } } } No its all true, I wish it wasn't but it is true. I have been a type } } } 1 Diabetic since 1963. Check out Diabetes and its long term complications. } } } I didn't mention it but I have also been diagnosed with the start of renal } } } kidney failure. I am on a vegetarian diet to slow down the failure rate } } and } } } with a couple of pills it has slowed down. I also didn't mention a bad } } } sprain that I did about 5 months ago that didn't heal and stayed swollen } } } and the foot doctor said this has caused the calcium to be leached out of } } } my foot so he has had me on crutches for the past two months until the } } foot } } } heals and the bones in my foot recalcifly. } } } I posted this in reply to a question about lasic surgery and meant } } } to encourage the questioner to do what he needed to do. Really the fact } } } that I work with microscopes has been a plus since I have been able to } } make } } } up for my eye problems and still do my job to my bosses satisfaction. With } } } a lot of other jobs I would have been out of work. } } } No Joke } } } Terry Ellis } } } } } } } } } } } } }
I have had good results doing immuno on Epon-Araldite embedded tissue by etching the plastic with sodium metaperiodate using the method described in the article "Ultrastructural Localization of Antigenic Sites on Osmium-fixed Tissues Applying the Protein A-Gold Technique" by Bendayan and Zollinger as published in The Journal of Histochemistry and Cytochemistry, Vol 31:1, pp101-109, 1983.
Stacey Andringa {Stacey.Andringa-at-uc.edu} on 09/09/2002 07:17:58 AM
To: Microscopy-at-sparc5.microscopy.com cc: (bcc: Mannie Steglich/MDACC)
Does anyone have a method to de-plasticize sections in Spurr resin that can allow immunohist to be done on them? Thanks. Stacey Andringa
The HIROX HiScope makes 3-D discernable on a flat screen with only one eye by utilizing kineopsis instead of stereopsis. see http://www.hirox-usa.com
Bill Miller
At 10:32 AM 9/10/2002 -0400, Ron L'Herault wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Colleagues... After 20 some years calibrating SRM484,our VG HB-50A UHV SEM come to the end. We are planning to dismantle the this cold FE, UHV microscope. Does any University or non-profit organization want this baby (still function) for free? Please contact me.
Joseph Fu National Institute of Standards & Technology 100 Bureau drive Stop 8212 Gaithersburg, MD. 20899-8212 Tel: 301-975-3495 Fax: 301-869-0822 Email: jofu-at-nist.gov
I do not use Spur's so I don't know if this will work but I have had good results doing immuno on Epon-Araldite embedded tissue by etching the plastic with sodium metaperiodate using the method described in the article "Ultrastructural Localization of Antigenic Sites on Osmium-fixed Tissues Applying the Protein A-Gold Technique" by Bendayan and Zollinger as published in The Journal of Histochemistry and Cytochemistry, Vol 31:1, pp101-109, 1983.
Stacey Andringa {Stacey.Andringa-at-uc.edu} on 09/09/2002 07:17:58 AM
To: Microscopy-at-sparc5.microscopy.com cc: (bcc: Mannie Steglich/MDACC)
Does anyone have a method to de-plasticize sections in Spurr resin that can allow immunohist to be done on them? Thanks. Stacey Andringa
Stacey Andringa {Stacey.Andringa-at-uc.edu} on 09/09/2002 07:17:58 AM
To: Microscopy-at-sparc5.microscopy.com cc: (bcc: Mannie Steglich/MDACC)
Does anyone have a method to de-plasticize sections in Spurr resin that can allow immunohist to be done on them? Thanks. Stacey Andringa
My apologies to you and everyone else I may have offended. I truly did not mean to do that and thought someone was making light of a serious medical condition.
You must tell me what Hallmark needs an SEM for. I'm just awfully curious as to its' application in that business.
Peter
-----Original Message----- } From: Terry E Ellis [mailto:tellis2-at-hallmark.com] Sent: Tuesday, September 10, 2002 8:32 AM To: microscopy-at-sparc5.microscopy.com
Peter: No its all true, I wish it wasn't but it is true. I have been a type 1 Diabetic since 1963. Check out Diabetes and its long term complications. I didn't mention it but I have also been diagnosed with the start of renal kidney failure. I am on a vegetarian diet to slow down the failure rate and with a couple of pills it has slowed down. I also didn't mention a bad sprain that I did about 5 months ago that didn't heal and stayed swollen and the foot doctor said this has caused the calcium to be leached out of my foot so he has had me on crutches for the past two months until the foot heals and the bones in my foot recalcifly. I posted this in reply to a question about lasic surgery and meant to encourage the questioner to do what he needed to do. Really the fact that I work with microscopes has been a plus since I have been able to make up for my eye problems and still do my job to my bosses satisfaction. With a lot of other jobs I would have been out of work. No Joke Terry Ellis
TMC makes nice floating granite stable tables using the same principle as for their SEM stabilizing platforms.
These babies are HEAVY. The one I've used is about 6" thick....solid granite. Floats like a feather. Has an Olympus MX-50 confocal on it.
gary g.
At 08:10 PM 9/9/2002, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
I doubt that it is a joke as it sound entirely plausable. I have some friends who deal with numerous life threatening health problem on a daily basis, fortunately I'm not one of them. I'm not making light of Terry Ellis's eye issues but some of these people make this the short list of what can go wrong. I'm not sure the human body was built on sound engineering principles; sometimes it's a miracle that it works as well as it does for as long as it does.
Damian Neuberger double lung transplant recipient } } I hope this is not some notion of a joke. It's a bad subject to joke about. } This all sounds highly improbable. I doubt whether Ray Charles would have } this many issues with vision. } } PT } } My name is Terry Ellis I work for Hallmark Cards Inc. and I run their } SEM-EDX equipment and also use a metallurgical, stereo and regular } microscope for sample prep and various projects. I am a diabetic and have } had several eye problems and surgeries. } one, the Doctor used a laser several to tack down my retina this has } reduced my night vision some but hasn't affected my microscope use. } Two, I had a detached retina in one eye then a year later a blood } vessel burst in the other eye, both times the doctor used microsurgery to } remove the fluid in my eye and lasers to correct the problems. Thank } goodness I still can see fine with both eyes, I have had to use a hat and } dark glasses since the body fluid that replaced the old fluid gel is much } clearer and I am more sensitive to light, on the microscopes I just use } less light. } Three, I had to have the lenses in both eyes replaced due to } cataracts in them, one lenses for distance and the other lens for close-up, } I have set up the binocular microscopes for my eyes by setting one eye } piece in focus then setting the other eye piece, which has an separate } focus knob, in focus then I can use the microscopes focus knobs to bring } it all in focus, which means that no one else can use them but I have a } camera and monitor that I move and set up for each microscope when some one } else needs to see what I see. } Four, I developed glaucoma in one eye and another Doctor put in what } he called a valve in it to relieve the pressure. I have lost some vision in } that eye but have been able to adjust the binoculars so I can almost see as } good with the bad eye but I generally use just one eye since I tend to get } headaches when I use both a lot. } During the surgery's I could only see with one eye and my boss still } calls me the one eyed microscopist. } Terry Ellis } tellis2-at-hallmark.com } 816-545-6573 } } }
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Hello, This is a two part (unrelated) question: 1. Is there a good software package that will construct 3D images from TEM serial sections? 2. Is artificial z stretching of very small moderately bright flourescent spots common when 3D movies are rotated? We are getting elongated elipses from deconvolved images (0.2 um stage steps, proper OTF from PSF for 100X lens), rather than spheres.
Hello: A short list of stuff that I have been asked to do. I get asked this question a lot at meetings and such. When we owned a plating company I used metallurgical procedures and our metallurgical microscope to cross-section a lot of samples and to measure their thickness'. The samples that were to thin to measure on the microscope I used the SEM to measure the thickness., I also used the EDX system to determine the composition of the different plating layers and core materials on all the samples. I still do this on plated items that we now buy from outside companies. I also have used these procedures on different broken machine parts, plant support ( such as cooling tower tubes and sprinkler piping with holes in them ), embossing dyes etc. We make our own gravvure and flexo printing plates and I have used the SEM-EDX to determine what caused plating defects in the gravvure printing plates and to evaluate different materials and procedures used to make flexo plates. We have several paper, ink, adhesive and printing chemists and I have supported their work with the SEM-EDX and light microscopes. Papers - their coatings, fillings, and type of paper fibers all have had o be known to get them to print right the SEM-EDX has helped a lot.. Inks - have to be matched with the right papers and printing process and their shapes, sizes ( usually done by a different procedure ) and composition, the SEM-EDX has been able to help determine possible problems. I could go on a long time about papers, inks and printing but I better stop since I have been told that I can be boring about stuff most people don't care about. I also use the SEM-EDX to determine particle sizes and composition of employees dust exposure in manufacturing, and office areas. Government regulations require special equipment when particle sizes fall below 10 microns. I also get samples of unknown bags of powder from all over - what it is type of questions. My favorite samples are white stuff scraped from around bathroom stools in hotels and plants that we are responsible for, although oversprayed paint on cars parked in our parking lots are cool too.
Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (kmccourt-at-NRCan.gc.ca) from http://www.msa.microscopy.com/Ask-A-Microscopist.html on Wednesday, September 11, 2002 at 12:08:12 ---------------------------------------------------------------------------
Email: kmccourt-at-NRCan.gc.ca Name: Stuart McCourt
Organization: Carleton University
Education: Undergraduate College
Location: Ottawa, Ontario Canada
Question: I am writing this for my son. We have an Olympus BHB microscope. We have been trying to get the manuals for this instrument but so far no luck. We have may questions. Que. there is a lens mounted below the condenser that moves with the condensor and plugs into the microscope. What is it for and when should it be used? Que. I have been told that the BHB uses short barrel objective lens not long barrel since I have lenses from a Wild microscope on it and they do not work correctly how do I know which lens to obtain? Que the microscope has a phase contrast unit again what objectives should I be looking at getting? I am looking a gettting a dark feild condenser will other dark feild condensers work if they fit into the condenser holder?
Remember we are microscopists too so we enjoy the boring stuff MOST people don't care about. I did a lot of work at the university i used to work at looking at paper. The art conservation students had old paper with neat paints and i got to find out what stuff the used for dyes and pigments. It was way cool.
Paul D. Nolan Electron Optics
Alcan International Limited Kingston Research and Development Centre P.O.Box 8400, 945 Princess Street Kingston, Ontario K7L 5L9
"Terry E Ellis" {tellis2-at-hallmar To: microscopy-at-sparc5.microscopy.com k.com} cc: Subject: What Hallmark does with SEM-EDX? 09/11/02 09:55 AM
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snip
I could go on a long time about papers, inks and printing but I better stop since I have been told that I can be boring about stuff most people don't care about.
Please do not contact me about this position, but follow the instructions below.
Nancy Phillips
Hewlett-Packard Company
The Hewlett-Packard company is a leading global provider of computing and imaging solutions and services for businesses and homes. The company focuses on capitalizating on the opportunities of the Internet and the proliferation of electronic services. HP has 85,400 employees worldwide in 120 countries. The total revenue from continuing operations was $42,5 billion in the 1999 fiscal year. For detailed information about HP, its products and services can be found on the World Wide Web at http://www.hp.com.
HP is an equal opportunity employer dedicated to affirmative action and workforce diversity. For more information about employment opportunities at HP, visit http://jobs.hp.com
Job Number : 810270 Job Title : TEM Engineer Department : Research & Development
United States : Oregon - Corvallis
Job Description:
In this job you will be working in an analytical laboratory within an HP development site. We have a world-class analytical laboratory with a wide variety of equipment. Our purpose is to support our HP Inkjet and emerging business partners with world-class analytical information to help solve complex materials, process, and product issues.
This is a Transmission Electron Microscopy (TEM) engineering position to work with a new state of the art TEM w/Field Emission, EDS, PEELS, and dual beam FIB sample preparation facilities. You will be developing and applying TEM, EELS, and other related applications as assigned. This will involve client consultations, sample preparation, running analysis on the appropriate tool/s, interpreting the results, providing a written report to the client with a review, lead or work in project teams delivering and documenting new applications or technologies. You will also be expected to serve as the primary TEM technical contact and develop working partnerships with other departments within the organization and HP. At times you will be asked to lead teams for initiating and developing existing and/or new technology. You will be expected to use statistical concepts to develop and execute experiments to support R&D and manufacturing, and maintain current knowledge of technology trends and developments in the Electron Microscopy community, specifically as this applies to TEM techniques.
Minimum Qualification :
Ph.D in Material Science, Physics, or related disciplines.
Experience includes: two-five years TEM experience including but not limited to: STEM, EELS (GIF, EFTEM), EDS, and Diffraction studies. With experience on semiconductors, metals, polymers, ceramics, in the form of bulk, thinfilms, and single crystals using a variety of sample prep techniques including FIB. Ultramicrotomy experience desired. General knowledge of SEM/EDS, Light Microscopy, XRD, Low dose EM and Tomography, and other analytical techniques. Ability to think outside the analytical box, good communicator, advanced computer skills, and self-motivated.
How do you apply ?
The quickest and most efficient way for us to process your resume is that you submit your resume to Hewlett-Packard by using the on-line application form. You will easily find the application form on http//www.jobs.hp.com.
please include the specific job ID number 810270 on top of your resume, or in your cover letter when applying for this function. If your interest in Hewlett-Packard was instigated by either a recruitment event or an advertisement, you should also include the specific event ID# (if it was provided to you at the event) or the advertisement ID#.. An advertisement ID# is typically part of the text within the Ad.
For information about additional job opportunities at HP, we recommend you use our on-line keyword search engine.This tool is available on http://www.jobs.hp.com You will be contacted if your resume fits the current position(s).If not, your application is put into a central database, accessible by any manager location. Each time we have a job opening, your information will be checked to see if it matches the requirements for the open positions. Your information will remain on our central database for six months. This means that you will only have to apply to us every six months. (You will be contacted if your resume fits the current position(s).If not, your application is put into a central database, accessible by any manager location).
To all; I forgot - from Hallmarks perspective we can protect our trade secrets and patents from disclosure or discovery and can control the timing of when the projects need to be done based on production needs. Terry
Training of new users is an interesting work. During the past year since I moved to the Texas A&M, I have been training more than a dozen new users of graduate students, undergraduate students and postdocs on the JEOL 2010 TEM. My experience is to keep the training as simple as possible.
In the beginning, in order to let the new users have a basic TEM theoretical background, they are required to read some chapters and respond to a questionnaire. Then for the hands-on training, I use a simple protocol to follow up and work with the new users until they feel comfortable working alone. Usually only about 5 sessions are needed for a new user. While I still keep myself available to assist them to solve some particular problems.
Since such a training is simple and the users are only responsible for few things to do with the operation, I get more and more users with the microscope.
Best regards,
Zhiping Luo Research Scientist Microscopy and Imaging Center, BSBW Texas A&M University, College Station, TX 77843-2257 Phone: (979) 845-1129 FAX: (979) 847-8933 E-mail: luo-at-mic.tamu.edu http://www.tamu.edu/mic
For the 3-D reconstruction, you could try Volocity™ (Version 1.4.1, Improvision). We used it succesfully to produce 3-D images of Toxoplasma Gondii parasites (Ref.: Nature 2002 Aug 1;418(6897):548-52 - check the movies in the supplemental materials).
The software is for use mainly with confocal light microscopy, but can be adapted easily for EM. It is quite expensive (} 20K), so only worth it if you intend to use it a lot.
Best
Marc
Mike Delannoy wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } Hello, } This is a two part (unrelated) question: } 1. Is there a good software package that will construct 3D images } from TEM serial sections? } 2. Is artificial z stretching of very small moderately bright } flourescent spots common when 3D movies are rotated? We are } getting elongated elipses from deconvolved images (0.2 um } stage steps, proper OTF from PSF for 100X lens), rather than } spheres. } } Thanks, } Mike D.
-- Marc Pypaert Department of Cell Biology, Center for Cell and Molecular Imaging and Ludwig Institute for Cancer Research, Yale University School of Medicine 333 Cedar Street New Haven CT 06520 Tel : (203) 785 3681 Fax : (203) 785 7446
Thank you for the explanation. Today I can say I learned something.
Peter
-----Original Message----- } From: Terry E Ellis [mailto:tellis2-at-hallmark.com] Sent: Wednesday, September 11, 2002 9:55 AM To: microscopy-at-sparc5.microscopy.com
Hello: A short list of stuff that I have been asked to do. I get asked this question a lot at meetings and such. When we owned a plating company I used metallurgical procedures and our metallurgical microscope to cross-section a lot of samples and to measure their thickness'. The samples that were to thin to measure on the microscope I used the SEM to measure the thickness., I also used the EDX system to determine the composition of the different plating layers and core materials on all the samples. I still do this on plated items that we now buy from outside companies. I also have used these procedures on different broken machine parts, plant support ( such as cooling tower tubes and sprinkler piping with holes in them ), embossing dyes etc. We make our own gravvure and flexo printing plates and I have used the SEM-EDX to determine what caused plating defects in the gravvure printing plates and to evaluate different materials and procedures used to make flexo plates. We have several paper, ink, adhesive and printing chemists and I have supported their work with the SEM-EDX and light microscopes. Papers - their coatings, fillings, and type of paper fibers all have had o be known to get them to print right the SEM-EDX has helped a lot.. Inks - have to be matched with the right papers and printing process and their shapes, sizes ( usually done by a different procedure ) and composition, the SEM-EDX has been able to help determine possible problems. I could go on a long time about papers, inks and printing but I better stop since I have been told that I can be boring about stuff most people don't care about. I also use the SEM-EDX to determine particle sizes and composition of employees dust exposure in manufacturing, and office areas. Government regulations require special equipment when particle sizes fall below 10 microns. I also get samples of unknown bags of powder from all over - what it is type of questions. My favorite samples are white stuff scraped from around bathroom stools in hotels and plants that we are responsible for, although oversprayed paint on cars parked in our parking lots are cool too.
Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (alicia.ortega-at-colorado.edu) from http://www.msa.microscopy.com/Ask-A-Microscopist.html on Wednesday, September 11, 2002 at 22:14:48 ---------------------------------------------------------------------------
Question: I have been trying to etch samples of polycrystalline NiTi to bring out grain boundaries so I can determine the grain size. Before etching I have been preparing the samples by polishing them down to a 0.25 micon diamond paste. The etchant I am using is 3HNO3+2H2O+1HF.
I tried leaving the etchant on for anywhere from 1 sec to 2 min, but nothing seems to work. I was wondering if anyine knows about or has any experience with ethcing NiTi and might know how long this particular etchant should take?
I am looking to buy JEOL used SEM & TEM. If you know of any good used 840,845,848, or newer SEM or 1200 EX , 1010, 2000 JEOL TEM or STEM please contact Dan at.
Daniel F. Connors 321-726-0669 321-544-5754 danieleds-at-aol.com
Hi, Does anyone out there uses Avalon 8000 or Spirit system by PGT? I am trying to get some positives and negatives about the systems. Or any other suggested systems that have EDS, Digital Imaging, X-ray mapping, pc based. The upgrade for Amray 1830I with EDS and WDS detectors.
Greetings Mike, Regarding your first question; the IMOD software package comes to mind (http://bio3d.colorado.edu/imod/). It is a free software package developed for SGI UNIX which has also been ported to Linux (standard PC hardware) and probably compiles on other UNIX platforms also. A place to look for other UNIX/Linux based freeware/shareware solutions for processing multidimensional data sets is http://www.cs.ubc.ca/spider/ladic/software.html. MS Windows native solutions tend to be proprietary (VoxBlast is one package which comes to mind), and I'm not familiar with most of them, although I believe ImageJ has some image alignment algorithm plugins, and it has a number of stack manipulation utilities. Once the images are aligned, the stack can be processed to a number of formats depending on what is required by your volume rendering software. Artificial stretching of spherical fluorescent sources in the z-axis can arise from a number of sources. The first thing that comes to mind is the point spread function--if the sample in question is mounted in a media with a refractive index significantly different from that which the point spread function was determined with then spherical abberation may distort the resultant image. Another source of distortion can be the fluorescent sphere itself-if the sphere is large enough, and is composed of a material of a refractive index different from the surrounding media, the fluorescent bead can act like a ball lens and weird images result. Hardware can always be a culprit. If the stage position feedback is encoded by the stepper motor only then it is difficult to tell how much the stage is really moving. In other words, if the stepper recieves a signal to move 2microns, and it turns 2 microns but the coupling to the stage z rack slips, then the stage just moved less than it was supposed to. On a couple of our microscopes the focus drive is actually a bearing friction coupling and it is capable of slipping. The computer, however, thinks the stage moved the correct distance, so the spacing between successive images in a stack is off. So if the computer thinks it moved 8 microns but it only really moved 6 microns then the image will be stretched. If a linear encoder is providing feedback to the software this problem should be minimized. Lastly, the rendering software needs to have the correct information-if the spacing between individual images in a stack is somehow entered incorrectly, the voxels may be stretched. Hope this helps. Regards, Karl G.
At 09:45 AM 9/11/2002 -0400, Mike Delannoy wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
_______________________________________________ Karl Garsha Light Microscopy Specialist Imaging Technology Group Beckman Institute for Advanced Science and Technology University of Illiniois at Urbana-Champaign 405 North Mathews Avenue Urbana, IL 61801 Room B650J Tel: (217) 244-6292 Fax: (217) 244-6219 www.itg.uiuc.edu
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Mike -
I downloaded the demo version of "3-D Doctor" but haven't yet had time to try it out on my images. You might want to look at their website and see if it looks promising for your work. I think the software package runs about $5000. http://www.ablesw.com/3d-doctor
Other sites that might be of interest (again I haven't had time to check these out): http://bio3d.colorado.edu/imod/ IMOD - freeware works in LINUX or on Silicon Graphics computer www.isi.uu.nl/people/michael/vr.htm VolumeJ - freeware Java (multiplatform, Windows compatible)
Neither I nor the company I work for have any financial interest in any of the above. I've just been looking around for ways to do reconstructions.
- Louise
Louise Harner Research Microscopist Albany International Research Co. 777 West Street, P.O. Box 9114 Mansfield, MA 02048 508-339-7300 phone 508-339-4996 fax Louise_Harner-at-albint.com
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Hello, This is a two part (unrelated) question: 1. Is there a good software package that will construct 3D images from TEM serial sections? 2. Is artificial z stretching of very small moderately bright flourescent spots common when 3D movies are rotated? We are getting elongated elipses from deconvolved images (0.2 um stage steps, proper OTF from PSF for 100X lens), rather than spheres.
Dear List, I will be purchasing a high-pressure freezer. I know that Balzers makes one, but I do not know whether there are other vendors. If anyone (including/especially vendors) has experience with either Balzers or other brands of high-pressure freezer, would you please contact me off-list? TIA. Yours, Bill Tivol
Can anyone suggest an independent service engineer who could perform a routine maintenance/PM on our Philips EM 300 (we are located just east of New York City on Long Island)? The scope is currently down with vacuum problem that I believe is related to poor water circulation (I have cleaned out a couple of filters in the plumbing down behind the panel in the front leg space of the scope without success). It should be noted that our greatest problem with service personnel is the Nassau County requirement that the individual carry $1,000,000 in liability insurance in order to work on campus.
Please contact me offline if you have any leads!
Regards,
Steve
Stephen J. Beck Associate Professor Bio-Imaging Center/Electron Microscopy Department of Biology Nassau Community College Garden City, NY 11530 Voice Mail: (516) 572-7829 Email: {becks-at-sunynassau.edu} URL: {http://www.sunynassau.edu/webpages/biology/becks.htm}
we have some problems with electromagnetic AC and DC fields in the room where our JEOL 2010F is installed. Therefore, I am currently looking into field cancellation systems. Installation of a Helmholtz cage has been recommended by the company who initially did the site survey. I would like to hear about any user's experience (positive and negative) with it and possible alternatives. I would be especially interested, if such a system can deal with interference from multiple and changing fields. Any advice/comment on this would be greatly appreciated, please contact me off-line if appropriate. Vendors suggestions are also welcome.
We etch NiTi alloys with a solution of 10 ml HF, 25 ml HNO3, and 150 ml water. Etching time is 15 to 30 sec. I suspect that your solution may be more uniformly dissolving the alloy without delineating the structure. Also, you should etch this alloy very quickly after polishing. Natural passivation will inhibit etching if you delay too long between final polish and etching. A fine oxide polish may also be needed to get a really good polish that will show a true structure.
Good luck. -- Larry D. Hanke, P.E. Materials Evaluation and Engineering, Inc. Practical Solutions Through Technology and Innovation http://www.mee-inc.com (763) 449-8870
You may want to dig into this more deeply. If I recall, the 1830i has integrated x-ray and does not support a separate system. There was some special thing done to PC10 frame buffer that caused this.
Make sure your SEM will accept a separate x-ray. If J9 is not used or if it has the External Beam Interface plate installed, you might have a chance.
gary
At 05:51 AM 9/12/2002, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
if you are intrested in trying our analySIS software with the 3D module, please contact me offline. The module allows reconstruction from serial sections. Check our web site for more information.
mike
Michael Bode, Ph.D. Soft Imaging System Corp. 12596 West Bayaud Avenue Suite 300 Lakewood, CO 80228 =================================== phone: (888) FIND SIS (303) 234-9270 fax: (303) 234-9271 email: mailto:info-at-soft-imaging.com web: http://www.soft-imaging.com ===================================
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Hello, This is a two part (unrelated) question: 1. Is there a good software package that will construct 3D images from TEM serial sections? 2. Is artificial z stretching of very small moderately bright flourescent spots common when 3D movies are rotated? We are getting elongated elipses from deconvolved images (0.2 um stage steps, proper OTF from PSF for 100X lens), rather than spheres.
} } In a message dated Thu, 5 Sep 2002 20:48:49 +1000, adavis-at-saipan.com writes: } } } } } As we enjoy great advantages from the inventions of others we should } } } be glad of an opportunity to serve others by any invention } } } of } } } ours, and this we should do freely and generously. } } } -- Benjamin Franklin } } } } } } } Alan- } } I'll start out by saying that Benjamin Franklin solved the } } controversy over patenting DNA sequences by major pharmaceutical } } firms and research companies. These companies point out that they } } have spent millions in research and want to make proprietary their } } DNA sequence results. I've always said, as did Franklin here, that } } the hundred years of scientific research, and all of the government } } funding and grants that laid the foundations of microbiology were } } accessed at no cost by the pharmaceutical companies and research } } companies. Should they not pay the estates of Pasteur, Koch, Semmelweis, and } } Lister, as well as Rosalind Carter who died of cancer from her work } } in x-ray crystallography to discover the DNA molecule? Many people } } contributed to the eventual result published by Watson and Crick- } } those who weighed the 4 bases that comprise DNA, those who } } determined it's components. Ben Franklin had it right. I have no } } problem with pharmaceutical companies or private research companies } } c! } harging as much as they want for the products of their research- but } they ought not restrict the knowledge. } } } } Now- about a flash unit in base. Easiest way is to get a small } } mirror and rig it just above the light in the base. Mount your } } flash pointed at it, and trip it via camera or manually. If the } } mirror is small enough, you'll still get enough light from the } } base-lamp up through the condenser to focus and compose the shot. } } The flash (set it on auto) will give you what you need on the film. } } If you want to see how I did mine- look at } } http://members.aol.com/moresciencestuff/microstuff.html } } bottom of the page. } } } } Good luck- } } Mike Shaw } } New Jersey
Dear Listers, I am interested in any information concerning darkroomless processing of 4489 EM film. I know of 2 processors on the market-one stand alone and the other water connected. Your knowledge and input on automated film processing of 4489 film is much appreciated.
Actually, the name was not Carter, it was Franklin.
Roger Moretz -- Where the world is only slightly less weird than it actually is. } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } } } In a message dated Thu, 5 Sep 2002 20:48:49 +1000, adavis-at-saipan.com writes: } } } } } } } As we enjoy great advantages from the inventions of others we should } } } } be glad of an opportunity to serve others by any invention } } } } of } } } } ours, and this we should do freely and generously. } } } } -- Benjamin Franklin } } } } } } } } } } Alan- } } } I'll start out by saying that Benjamin Franklin solved the } } } controversy over patenting DNA sequences by major pharmaceutical } } } firms and research companies. These companies point out that they } } } have spent millions in research and want to make proprietary their } } } DNA sequence results. I've always said, as did Franklin here, that } } } the hundred years of scientific research, and all of the government } } } funding and grants that laid the foundations of microbiology were } } } accessed at no cost by the pharmaceutical companies and research } } } companies. Should they not pay the estates of Pasteur, Koch, Semmelweis, and } } } Lister, as well as Rosalind Carter who died of cancer from her work } } } in x-ray crystallography to discover the DNA molecule? Many people } } } contributed to the eventual result published by Watson and Crick- } } } those who weighed the 4 bases that comprise DNA, those who } } } determined it's components. Ben Franklin had it right. I have no } } } problem with pharmaceutical companies or private research companies } } } c! } } harging as much as they want for the products of their research- but } } they ought not restrict the knowledge. } } } } } } Now- about a flash unit in base. Easiest way is to get a small } } } mirror and rig it just above the light in the base. Mount your } } } flash pointed at it, and trip it via camera or manually. If the } } } mirror is small enough, you'll still get enough light from the } } } base-lamp up through the condenser to focus and compose the shot. } } } The flash (set it on auto) will give you what you need on the film. } } } If you want to see how I did mine- look at } } } http://members.aol.com/moresciencestuff/microstuff.html } } } bottom of the page. } } } } } } Good luck- } } } Mike Shaw } } } New Jersey }
Hello, Does anyone offer service for a Leitz Aristoplan on the West Coast? We have an Aristoplan with the Variophot photohead that generates its own dirt and haze in the sealed optics, and needs the focus re-lubed. I'm tired of shipping it to Leica in New Jersey just to have the internal surfaces lined with thumbprints and new dirt to replace the old.
Regards, glen -- Glen MacDonald Microscopy and Imaging Facility University of Washington Core for Communication Research Virginia Merrill Bloedel Hearing Research Center Box 357923 University of Washington Seattle, WA 98195-7923 glenmac-at-u.washington.edu (206) 616-4156 (206) 616-1828 fax ************************************************************************** C:} The box said "Requires Windows95 or better". So I bought a Macintosh. **************************************************************************
I have an uneven field of illumination in my microscope when I do bright field microscopy. I have tried to align the bulb to even out the field but I am not having much luck. I am using 20x and 63x Plan Apo objectives and the scope is in "perfect" Kohler illumination. I know how to subtract this variation with image processing but it would obviously be better to minimize this variation in the original. What I am wondering is how much variability should I expect in a well aligned, clean microscope? If one takes a digital image of a blank field using either a 20x 0.5 NA objective or a 63x PlanApo oil NA 1.25 objective, how wide of a pixel intensity would you find acceptable? Is there something I should be concerned with other than the bulb alignment? TIA, Tom
-- Thomas E. Phillips, Ph.D. Associate Professor of Biological Sciences Director, Molecular Cytology Core Facility
3 Tucker Hall Division of Biological Sciences University of Missouri Columbia, MO 65211-7400 (573)-882-4712 (voice) (573)-882-0123 (fax)
Dear Listers, I am interested in any information concerning darkroomless processing of 4489 EM film. I know of 2 contained, auto processors on the market-one stand alone and the other water connected. Your knowledge and input on automated film processing of 4489 film will be appreciated.
I'm trying to find a commercial source of goat anti-chicken (serum proteins, not egg) antibody conjugated to 10 nm gold particles. I would deeply appreciate any recommendations anyone can give me. If you have personal knowledge of the product's quality, that would be even better, but not necessary--at this point, I'm just trying to find out who offers it.
Thank you,
Margaret Dienelt
Plant Pathologist/Electron Microscopist
Floral and Nursery Plants Research Unit National Arboretum Agricultural Research Service, USDA
Beltsville Agriculural Research Center Bldg. 010A Rm. 248 10300 Baltimore Avenue Beltsville Maryland 20705
I would like to forword this entire email to members of a legal list server regards copyrights and patents.
Who that has the authority could give me permission to do?
also from where did the Franklin quote originate? sterling
On Fri, 13 Sep 2002 rcmoretz-at-att.net-at-sparc5.microscopy.com wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Actually, the name was not Carter, it was Franklin. } } Roger Moretz } -- } Where the world is only slightly } less weird than it actually is. } } ------------------------------------------------------------------------ } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } } -----------------------------------------------------------------------. } } } } } } } } In a message dated Thu, 5 Sep 2002 20:48:49 +1000, adavis-at-saipan.com writes: } } } } } } } } } As we enjoy great advantages from the inventions of others we should } } } } } be glad of an opportunity to serve others by any invention } } } } } of } } } } } ours, and this we should do freely and generously. } } } } } -- Benjamin Franklin } } } } } } } } } } } } } Alan- } } } } I'll start out by saying that Benjamin Franklin solved the } } } } controversy over patenting DNA sequences by major pharmaceutical } } } } firms and research companies. These companies point out that they } } } } have spent millions in research and want to make proprietary their } } } } DNA sequence results. I've always said, as did Franklin here, that } } } } the hundred years of scientific research, and all of the government } } } } funding and grants that laid the foundations of microbiology were } } } } accessed at no cost by the pharmaceutical companies and research } } } } companies. Should they not pay the estates of Pasteur, Koch, Semmelweis, and } } } } Lister, as well as Rosalind Carter who died of cancer from her work } } } } in x-ray crystallography to discover the DNA molecule? Many people } } } } contributed to the eventual result published by Watson and Crick- } } } } those who weighed the 4 bases that comprise DNA, those who } } } } determined it's components. Ben Franklin had it right. I have no } } } } problem with pharmaceutical companies or private research companies } } } } c! } } } harging as much as they want for the products of their research- but } } } they ought not restrict the knowledge. } } } } } } } } Now- about a flash unit in base. Easiest way is to get a small } } } } mirror and rig it just above the light in the base. Mount your } } } } flash pointed at it, and trip it via camera or manually. If the } } } } mirror is small enough, you'll still get enough light from the } } } } base-lamp up through the condenser to focus and compose the shot. } } } } The flash (set it on auto) will give you what you need on the film. } } } } If you want to see how I did mine- look at } } } } http://members.aol.com/moresciencestuff/microstuff.html } } } } bottom of the page. } } } } } } } } Good luck- } } } } Mike Shaw } } } } New Jersey } } }
I was told that at this past M&M meeting, both Hitachi and JEOL demonstrated their newest FESEM models - Hitachi S-4800 and JSM-7400F. I was wondering if any of you could make comments concerning these two or other FESEM versions. I'm especially interested in the quality of corresponding cold FEGs, data base management, and proprietary technologies such as ExB, energy filter, and in-lens or semi in-lens detectors. Both on and off line responses are welcome. Thanks in advance!
**************************************** Chaoying Ni The W.M. Keck Electron Microscopy Facility College of Engineering University of Delaware Newark, DE 19716
On our recently installed FETEM, I have noticed that when the magnification is x800k-1.5M, the beam crossover loses its smoothness of the edge. The shape also becomes off-circular. The alignment doesn't seem to be an issue (checked both by myself and service engineer). My question is whether this is normal or acceptable (scope is still under warranty). Can anyone shed some light on this? Thanks!
**************************************** Chaoying Ni The W.M. Keck Electron Microscopy Facility College of Engineering University of Delaware Newark, DE 19716
Dear Luc It was pleasure to be at ICEM-15. I was impressed how well everything were organized and program was great. Thanks! Sergey
At 03:43 PM 9/10/02 +0200, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Sergey Ryazantsev, Ph.D. Electron Microscopy Department of Biological Chemistry, School of Medicine University of California, Los Angeles Box 951737 Los Angeles, CA 90095-1737
I am not an expert in this area, but just completed Cryo-EM course and had chance to work on Balzers and Leica's instruments. Leica's is compact, use a fraction of LN2 Balzers used and more easy to operate. Could not say anything about sample's quality - I could not get them from Elanie for a few month. I would suggest you ask for demo and compare results side-by-side. Best wishes, Sergey
} Date: Thu, 12 Sep 2002 11:00:44 -0400 } From: Bill & Sue Tivol {wtivol-at-earthlink.net} } Subject: High-pressure freezer vendors } To: microscopy list {microscopy-at-sparc5.microscopy.com} } User-Agent: Microsoft Outlook Express Macintosh Edition - 5.01 (1630) } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Such distortion of the beam is usually caused by charging of contaminants on the surface of the condenser aperture. Changing or cleaning the aperture may help. When the beam diameter is very small (like the one needed for the magnification range you mentioned) such roughness of the beam edge is considered normal. Try switching the condenser apertures and see if there is big difference in the beam shape between different apertures. If one of the apertures is "dirty" there will be big difference in distortion between it and the other apertures. If all the apertures show comparable roughness - don't bother to change or clean them ... the situation may worsen. The problem of condenser aperture charging is much more severe for FEG than LaB6 guns. The FEG is much brighter source producing very small crossover (high coherency). If you were using LaB6 in the magnification range you mention you'll usually work with the beam in crossover.
Hope this helps.
Best regards,
Rado
--------------------------------------------------------------------- Radostin Danev, Ph.D. Laboratory of Ultrastructure Research National Institute for Physiological Sciences Myodaiji-cho, Okazaki 444-8585, JAPAN phone: 0564-55-7813 e-mail: rado-at-nips.ac.jp ---------------------------------------------------------------------
----- Original Message ----- } From: "Chaoying Ni" {cni-at-udel.edu} To: {Microscopy-at-sparc5.microscopy.com} Sent: Saturday, September 14, 2002 10:52 PM
Have you considered Otto Breiner Instruments? He's well known here in the Detroit area. Here's the business card information:
246 Heather Heights Monrovia, CA 91016 ph 818-357-3859 fax 818-358-1209
Stu Smalinskas SKF North American Technical Center Plymouth, Michigan
__________________________________________________ Do You Yahoo!? Yahoo! Finance - Get real-time stock quotes http://finance.yahoo.com
Hi Margaret, You will find donkey anti-chicken IgY (H+L) conjugated to gold at Bio/Can Scientific (Jackson Immunoresearch); they have 6, 12 and 18 nm gold conjugates. You can reach them at one of these numbers: 800-367-5296; 610-869-4024; 800-387-8125; or websites: www.jacksonimmuno.com or www.biocan.com I haven't use those so I can't tell you much more than that. Good luck! Emmanuelle
Postdoctoral Fellow or Research Associate - Morphology Core
The Buck Institute for Age Research aims to increase the healthy years of life through clinically relevant biomedical research on the biology of aging and age-associated diseases. Established as an independent, nonprofit research facility, the Buck Institute is located in Marin County north of the San Francisco and brings a new focus to the science of aging with a world-class Faculty.
Candidates with a strong commitment to understanding aging and the causes of age-related disease are sought for the technical position of a Postdoctoral Fellow or Research Associate to join its Morphology Core facility. Duties will include sample preparation using basic histology and immunochemistry techniques, image analysis, and minor equipment maintenance. Successful candidate will instruct and assist the users of the facility and will actively participate in the ongoing research projects. Applicants should have experience in the basic histology/immunocytochemistry, fluorescence and transmitted light microscopy, and some image analysis. Experience in electron microscopy will be a plus. Excellent communication and organizational skills and the ability to manage a large workload are a must. Salary will depend upon qualification and experience. Some training will be provided. We offer a competitive salary, excellent benefits, dynamic work environment, and new state-of-the-art facility. To apply, send cover letter and resume with MC/RA on the subject line of the e-mail, to hr-at-buckinstitute.org You are welcome to contact me if you have any questions about this position.
Anna Logvinova, M.D. Morphology Core Manager Buck Institute 8001 Redwood Blvd Novato, CA 94948 www.buckinstitute.org
I run the core EM facility at UNMC in Omaha, NE. and I would like to set up some sort of teleconferencing or telemicroscopy link with the local biology classes. The teachers and myself of course have no experience in this. I would like to hear from anyone who has been involved in this sort of arrangement. All help and advice will be greatly appreciated.
Dear Chris To test/calibrate my laser diffractometer I used to use copper/nickel 150-300 mesh sheets. We used that material, also, to punch 3 mm EM grids in the early era of EM. Originally it comes from electronic industry where used in 'magnetron' production. You probably could obtain similar material from EM grids suppliers (may be expensive if special order). You could print such 'mesh' by contact printing on hi-res film. Such sample delivered very nice diffraction pattern. It's not such funny as Esher figures but nice test-sample for laser diffractometer. Another idea: to use old friend - protection technique. Make Hi-res print-out of your funny images, use conventional film enlarger in 'opposite' way: load unexposed film in the film-holder and project your print-out on the film. It'll take some experimenting with focusing, illumination, exposure etc. You may also use convention SLR 35mm camera with hi-res/hi contrast sci grade film to take pictures. Your drawings should be large enough. I think, it's simplest way to do so. If need details, you may contact me off-line. Good luck, Sergey.
At 08:58 AM 9/3/02 +0100, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Sergey Ryazantsev, Ph.D. Electron Microscopy Department of Biological Chemistry, School of Medicine University of California, Los Angeles Box 951737 Los Angeles, CA 90095-1737
I am interested in purchasing a scanner as a back-up in the event our CCD camera should fail or to scan old 3 1/4 x 4 negatives, if necessary. We have a Philips EM208S TEM and an AMT 2K CCD camera. I have checked on the Agfa Duoscan and found that it is no longer in production. Is anyone using another reasonably priced scanner and if so, which one? Any information would be greatly appreciated.
Thank-you.
Sharon Walsh System Technical Specialist Laboratory Sciences of Arizona Good Samaritan Medical Center Phoenix, Az. (602)239-2343
} I am interested in purchasing a scanner as a back-up in the event our CCD } camera should fail or to scan old 3 1/4 x 4 negatives, if necessary. We } have a Philips EM208S TEM and an AMT 2K CCD camera. I have checked on the } Agfa Duoscan and found that it is no longer in production. Is anyone } using another reasonably priced scanner and if so, which one? Any } information would be greatly appreciated. } } Thank-you. } } Sharon Walsh } System Technical Specialist } Laboratory Sciences of Arizona } Good Samaritan Medical Center } Phoenix, Az. } (602)239-2343
Check out the Nikon CoolScan 8000. It will just barely handle TEM negs. But will definitely handle 35mm and MF formats.
The Microtek Artixscan 2500f is the mechanical twin of the Agfa Duoscan T2500. It has been updated with both IEEE1394 (Firewire) and SCSI interfaces and an improved dynamic range. The carrier design, like the Duoscan is glassless. The 4x5 carrier works well to hold 3.25x4 TEM negs. We have a PDF I am happy to send or visit http://www.microtekusa.com/as2500f.html
The Artixscan 1100 has a similar design but with lower optical resolution and SCSI interface only. http://www.microtekusa.com/as2500f.html
We have customers very happy with both.
George
George Laing National Graphic Supply ph 800.223.7130 x3109 f 800.832.2205 email scisales-at-ngscorp.com
I am interested in purchasing a scanner as a back-up in the event our CCD camera should fail or to scan old 3 1/4 x 4 negatives, if necessary. We have a Philips EM208S TEM and an AMT 2K CCD camera. I have checked on the Agfa Duoscan and found that it is no longer in production. Is anyone using another reasonably priced scanner and if so, which one? Any information would be greatly appreciated.
Thank-you.
Sharon Walsh System Technical Specialist Laboratory Sciences of Arizona Good Samaritan Medical Center Phoenix, Az. (602)239-2343
I thought I'd send a message for a quick response (hopefully I don't get daggers thrown at me) - with respect to disposable lab coats. I was asked about the possibility of using them, for people coming into the lab to work on equipment, or visitors wanting to observe techniques. As part of the New Safety regulations, I have to make sure people have access to proper protective clothing. It has been argued that lab coats are contaminated when a person goes into our lab, because of the arsenic, and other contaminants we use. I know this question sounds a bit ridiculous to some, but it was suggested to me, that we have disposable lab coats for students, visitors, and any one else entering the lab.
Does anyone have any helpful thoughts on this, and could provide some helpful advice?
Thanks in advance,
Susan
Susan Carbyn Electron Microscopy Technician Atlantic Food and Horticulture Research Centre Agriculture and Agri-Food Canada 32 Main Street, Kentville, N.S. B4N 1J5 Canada
"Walsh, Sharon (by way of MicroscopyListserver)" wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } I am interested in purchasing a scanner as a back-up in the event our } CCD camera should fail or to scan old 3 1/4 x 4 negatives, if } necessary. We have a Philips EM208S TEM and an AMT 2K CCD camera. I } have checked on the Agfa Duoscan and found that it is no longer in } production. Is anyone using another reasonably priced scanner and if } so, which one? Any information would be greatly appreciated. } } Thank-you. } } Sharon Walsh } System Technical Specialist } Laboratory Sciences of Arizona } Good Samaritan Medical Center } Phoenix, Az. } (602)239-2343
Get an Epson 2450 with the transparency adapter. Does a great job for about $400. The Nikon 8000 (and Minolta Dimage Scan Multi Pro) will only do a 6cm x 9cm portion of a TEM negative.
Geoff -- ********************************************** Geoff McAuliffe, Ph.D. Neuroscience and Cell Biology Robert Wood Johnson Medical School 675 Hoes Lane, Piscataway, NJ 08854 voice: (732)-235-4583; fax: -4029 mcauliff-at-umdnj.edu **********************************************
I am a philosopher/historian of science/technology, with a particular interest in scientific instruments. I am now starting research into the history of the development of scanning tunneling microscopy and atomic force microscopy. I am interested in the range of issues that involve these developments, but I am particularly interested in (and having some difficulty finding information about) how various commercial instrument makers picked up and developed these technologies. Here I would like to know who did this, how they interacted with the academic and commercial research communities, and how innovations were exchanged between these interacting communities.
Thanks for whatever help members can provide.
Davis Baird -- ******************************************************************** Davis Baird db-at-sc.edu http://www.cla.sc.edu/PHIL/faculty/baird/INDEX.HTM Editor, Techne: Journal of the Society for Philosophy and Technology Professor and Chair Department of Philosophy University of South Carolina Columbia, SC 29208 USA (803) 777-4166 FAX (803) 777-9178 ********************************************************************
Microtek supply a whole range of glassless scanners of the Agfa duoscan type (i'm not sure if they just took over some of the Agfa Duoscan range).
The scanners of most interest to you are probably: Duoscan style with conventional flatbed and seperate glassless holders for up to about 5x10 or 8x10 inches (not cms) Microtek Scanmaker 8700 cheapest - comes as a basic model or PRO version with better software Microtek Artixscan 1100 Microtek Artixscan 2500f most expensive There are more but they seem to go up to A3 or do other things I don't want.
dedicated large format film scanner : (will take negatives up to 4x5 inches) Microtek Artixscan 4500t
All have some glassless holders and range from 1200 dpi up to 2500 dpi with Dmax from 3.4 up to 3.9; colour depth is 42 bit which should translate to 14 bit B&W. Interfaces vary from SCSI, USB and firewire. Prices appear to be from 600 UK pounds to 3,100 UK pounds.
You could start with the website at http://www.microtekusa.com (check out products and the 3 ranges of scanners) and perhaps run a search engine for more background information.
I don't have a Microtek at present and I have no connection with the company but I am probably going to get one of the cheaper ones. If anyone has any user experience of these scanners I would be interested in their opinions.
Good luck.
Malcolm Haswell E.M. Unit School of Health, Natural and Social Sciences University of Sunderland UK
"Walsh, Sharon (by way of MicroscopyListserver)" wrote: } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } I am interested in purchasing a scanner as a back-up in the event our } CCD camera should fail or to scan old 3 1/4 x 4 negatives, if } necessary. We have a Philips EM208S TEM and an AMT 2K CCD camera. I } have checked on the Agfa Duoscan and found that it is no longer in } production. Is anyone using another reasonably priced scanner and if } so, which one? Any information would be greatly appreciated. } } Thank-you. } } Sharon Walsh } System Technical Specialist } Laboratory Sciences of Arizona } Good Samaritan Medical Center } Phoenix, Az. } (602)239-2343
I recently posted a querry requesting a good source of adhesive for serial sections of plastic blocks.
I found that scotch tape dissolved in xylene works fine.
Thanks contributors, Tim Quinn University of Kansas Program Assistant/Microscopists/Lab Mgr Ornithology Dept. Natural History Museum and Biodiversity Research Center Dyche Hall Room 414 Lawrence, KS 6604-2454 785-864-4556/785-331-4107 tquinn-at-ku.edu
A invaluable source for finding antibodies is Linscott's Directory. Their address is 815 Whitney Way, Petaluma, CA 94954 (707-763-7098). http://www.linscottsdirectory.com
They list not only the antibodies, but where to order them. There is a fee for the catalog and/or the online directory. I highly recommend it.
Peggy
Peggy Sherwood Lab Associate, Photopathology Wellman Laboratories of Photomedicine (W224) Massachusetts General Hospital 55 Fruit Street Boston, MA 02114 617-724-4839 (voice mail) 617-726-6983 (lab) 617-726-3192 (fax) msherwood-at-partners.org
} -----Original Message----- } From: Margaret Brannigan [SMTP:brannign-at-asrr.arsusda.gov] } Sent: Friday, September 13, 2002 4:41 PM } To: Microscopy-at-sparc5.microscopy.com } Subject: TEM: Need gold conjugate source } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } } -- } Hi, } } I'm trying to find a commercial source of goat anti-chicken (serum } proteins, not egg) antibody conjugated to 10 nm gold particles. I } would deeply appreciate any recommendations anyone can give me. If } you have personal knowledge of the product's quality, that would be } even better, but not necessary--at this point, I'm just trying to } find out who offers it. } } Thank you, } } Margaret Dienelt } } Plant Pathologist/Electron Microscopist } } } Floral and Nursery Plants Research Unit } National Arboretum } Agricultural Research Service, USDA } } Beltsville Agriculural Research Center } Bldg. 010A Rm. 248 } 10300 Baltimore Avenue } Beltsville Maryland 20705 } } (301) 504-6097 }
} } } I am interested in purchasing a scanner as a back-up in the event } our CCD camera should fail or to scan old 3 1/4 x 4 negatives, if } necessary. We have a Philips EM208S TEM and an AMT 2K CCD camera. } I have checked on the Agfa Duoscan and found that it is no longer in } production. Is anyone using another reasonably priced scanner and } if so, which one? Any information would be greatly appreciated. } ***************
hi Sharon, I have an EPSONExpression 1600 Pro with a transilluminator. I have had good results with it. It has true optical resolution of 1600 dpi, was very easy to install (has Fire Wire, USB and SCSI2 interfaces). It was also VERY reasonably priced, which was good for me because I had $4500 with which to upgrade my whole computer/printer/scanner system. I does not have a film holder for EM plates, but it does have a focus adjustment to account for the film lying on the scanner bed and i have not had any trouble with moire lines, etc. I"m sure the more expensive scanners have better options/feature, but this was very good for its price. Lee
}
-- Leona Cohen-Gould, M.S. Sr. Staff Associate Director, Electron Microscopy Core Facility Manager, Optical Microscopy Core Facility Joan & Sanford I. Weill Medical College of Cornell University voice (212)746-6146 fax (212)746-8175
I like the Epson 1680 - it has a Dmax of 3.6 - you need the highest Dmax you can get when you are working with EM negatives. Remember this is a log scale so each 0.3 difference is 10x better. We scan in the 16 bit mode, then adjust levels using Photoshop and then convert to 8 bit so that we get max contrast range without all those annoying gaps between pixel densities.
-- Thomas E. Phillips, Ph.D. Associate Professor of Biological Sciences Director, Molecular Cytology Core Facility
3 Tucker Hall Division of Biological Sciences University of Missouri Columbia, MO 65211-7400 (573)-882-4712 (voice) (573)-882-0123 (fax)
I have a potential client who is looking to rent time on an ESEM (preferably) or SEM in the Dallas Fort Worth Texas (preferred) or Houston Texas area. He has a corroded copper plug ( { 1 inch in diameter) that he would like to get some EDS data on. If you are interested please reply off-line.
Thank you, James Talbot
K/T GeoServices, Inc. Bulk and Clay Mineralogy by X-ray Diffraction (940) 597-9076 web site: http://www.ktgeo.com/
I apologize is this is not strictly a microscopy question. A microscopist colleague/friend of mine is interested in purchasing a high quality speech recognition software. The individual is handicapped and does not full use of their hands and would be using the software for scientific writing (primarily describing microscopy findings). Although I favor the Macintosh system (since they would also use the computer for image processing and publishing), I am looking for the best software to assist this individual. Any recommendations would be appreciated. Many thanks.
JB
############################################################## John J. Bozzola, Ph.D., Director I.M.A.G.E. (Integrated Microscopy & Graphics Expertise) 750 Communications Drive - MC 4402 Southern Illinois University Carbondale, IL 62901 U.S.A. Phone: 618-453-3730 Fax: 618-453-2665 Email: bozzola-at-siu.edu Web: http://www.siu.edu/~image/ ##############################################################
We are forced to evaluate methods of improving efficiency of sample preparation in our TEM laboratory and would like to hear your opinions on the following semi-automated approaches. The lab processes nearly a 1000 TEM samples per year, mostly cross-sections of CMOS devices on Si wafers. We use manual polishing, dimpling, ion mills, and FIBs tools, however we don't have enough people to handle the load and will not see an increase in headcount in the near future. I would appreciate any and all input on the following combinations of methods and equipment.
* wafering saw and FIB
vs.
* semi-automated polisher and ion mill
vs.
* precision cleaving and FIB
Thank you in advance for your opinions and accounts of your experiences with those approaches.
Regards,
Jerzy
****************************************************** Jerzy Gazda, Ph.D. Advanced Micro Devices Supervising Engineer 5204 E. Ben White Blvd. - MS 613 PCAL - AIM Section Austin, TX 78741 TEL: 1-800-538-8450, Ext. 51453 FAX: (512) 602-7470 jerzy.gazda-at-amd.com ******************************************************
From root Tue Sep 17 17:47:07 2002 Return-Path: {Microscopy-request-at-sparc5.microscopy.com} Received: (from daemon-at-localhost) by sparc5.microscopy.com (8.9.3+Sun/8.9.3) id RAA14718 for dist-Microscopy; Tue, 17 Sep 2002 17:14:12 -0500 (CDT) Received: from njz_spm_filter (sparc5 [206.69.208.10]) by sparc5.microscopy.com (8.9.3+Sun/8.9.3) with SMTP id RAA14711 for "MicroscopyFilteredEmail1-at-msa.microscopy.com"; Tue, 17 Sep 2002 17:13:41 -0500 (CDT)
Dear Listers,
We are forced to evaluate methods of improving efficiency of sample preparation in our TEM laboratory and would like to hear your opinions on the following semi-automated approaches. The lab processes nearly a 1000 TEM samples per year, mostly cross-sections of CMOS devices on Si wafers. We use manual polishing, dimpling, ion mills, and FIBs tools, however we don't have enough people to handle the load and will not see an increase in headcount in the near future. I would appreciate any and all input on the following combinations of methods and equipment.
* wafering saw and FIB
vs.
* semi-automated polisher and ion mill
vs.
* precision cleaving and FIB
Thank you in advance for your opinions and accounts of your experiences with those approaches.
Regards,
Jerzy
****************************************************** Jerzy Gazda, Ph.D. Advanced Micro Devices Supervising Engineer 5204 E. Ben White Blvd. - MS 613 PCAL - AIM Section Austin, TX 78741 TEL: 1-800-538-8450, Ext. 51453 FAX: (512) 602-7470 jerzy.gazda-at-amd.com ******************************************************
Short of getting instruments that are pre-pared for remote, you can do the following.
Start at Oak Ridge to see the high end of your dreams.
http://www.ms.ornl.gov/htmlhome/mauc/default.htm
Then take a trip to BUGSCOPE:
http://bugscope.beckman.uiuc.edu/
And finally, stop off at the HOME of BugScope:
http://www.itg.uiuc.edu/technology/, where you can find other outreach programs to emulate.
Finally, finally, a real favorite, and a very worthwhile stop:
http://www.sci.sdsu.edu/EM_Facility/index.html
Hope this helps to answer some of your questions.
Regards,
Fred Monson
Frederick C. Monson, PhD Center for Advanced Scientific Imaging Schmucker II Science Center c/o Geology/Astronomy West Chester University South Church Street and Rosedale Ave West Chester, Pennsylvania, USA, 19383 Phone: 610-738-0437 FAX: 610-738-0437 fmonson-at-wcupa.edu CASI URL: http://darwin.wcupa.edu/casi/ WCUPA URL: http://www.wcupa.edu/ Visitors URL: http://www.wcupa.edu/_visitors/
THINKING IS MUCH MORE DIFFICULT THAN MEMORIZING.
} ---------- } From: "tbargar-at-unmc.edu"-at-sparc5.microscopy.com } Sent: Monday, September 16, 2002 2:01 PM } To: Microscopy-at-sparc5.microscopy.com } Subject: Telemicroscopy for the classroom } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } } } __________________ } } I run the core EM facility at UNMC in Omaha, NE. and I would like to set } up } some sort of teleconferencing or telemicroscopy link with the local } biology } classes. The teachers and myself of course have no experience in this. I } would like to hear from anyone who has been involved in this sort of } arrangement. All help and advice will be greatly appreciated. } } Tom Bargar } 402-559-7347 } tbargar-at-unmc.edu } } } }
This reply may not be relevant to your query, but I have recently found out how good current domestic flatbed scanners are.
I bought a CanoScan D1250UF, the F means it has a little fluorescent light built in to the lid, for scanning 35mm film/slides. Less than US$200.
The holder can easily accept two pieces of polaroid film as well as a standard petrological thinsection, and, with the thing set for 2400 dpi, in a few minutes (less, if your computer has USB-2), you have a digital image of the whole thinsection in transmitted light with crossed polars, at good enough quality to blowup to A4 size!
Sure makes it easy to find your way around when the thinsection is in the EPMA, bound to be other uses as well eg depicting textures.
cheers
rtch
} } I am interested in purchasing a scanner as a back-up in the event our } CCD camera should fail or to scan old 3 1/4 x 4 negatives, if } necessary. We have a Philips EM208S TEM and an AMT 2K CCD camera. I } have checked on the Agfa Duoscan and found that it is no longer in } production. Is anyone using another reasonably priced scanner and if } so, which one? Any information would be greatly appreciated. }
Ritchie Sims Phone : 64 9 3737599 ext 7713 Department of Geology Fax : 64 9 3737435 The University of Auckland email : r.sims-at-auckland.ac.nz Private Bag 92019 Auckland New Zealand
Hi Jerzy, we have a similar workload to you, but in III-V's (we have looked at 475 TEM samples since April 1). We have only 2 people (myself and one other) doing all the sample prep, TEM and report writing. Much of our work is straightforward thickness measurements and cross-sections, and we have no FIB.
Do you have a Gatan PIPS or similar low-angle ion mill, with the ability to mill from predominantly one direction? I've found a great way of making cross sections using this machine combined with precision(ish) cleaving, cutting out several stages from the 'standard' way of doing things. Typical InP cross sections take less than an hour to do; with the right kind of sample (i.e. not site specific in 2 dimensions) it is possible to stack them up and do up to 10 at a time. It's straightforward to hit features down to 20um in size, but if you want to keep the specimen you really have to do one at a time. (It's impossible to get several specific sites thin at the same time, meaning you have to look at the first region that becomes electron transparent, then destroy it while getting the next one thin, etc..) Si takes longer since it ion mills so much more slowly, but the few I've done still take less than 90 mins from getting the sample to looking at it in the TEM.
I've been thinking of writing this up and publishing it somewhere, since it has saved us a huge amount of time and effort. I'm sure that if you were working with Si all the time you'd be able to optimise the procedure still further. I'll try to get some words together describing the procedure, with pictures, if you like.
FIB is great for very specific sites (less than 10um or so, depending on the structure) and I do use one in a tame academic's lab every so often, but for fast cross sections with lots of thin area I can't beat 'standard' methods. However I appreciate that Si geometries are often several orders of magnitude smaller and more complex than III-Vs, and site specific samples are likely to be a much bigger proportion of your workload.
-----Original Message----- } From: "jerzy.gazda-at-amd.com"-at-sparc5.microscopy.com [mailto:"jerzy.gazda-at-amd.com"-at-sparc5.microscopy.com] Sent: 17 September 2002 23:09 To: Microscopy-at-sparc5.microscopy.com
Dear Listers,
We are forced to evaluate methods of improving efficiency of sample preparation in our TEM laboratory and would like to hear your opinions on the following semi-automated approaches. The lab processes nearly a 1000 TEM samples per year, mostly cross-sections of CMOS devices on Si wafers. We use manual polishing, dimpling, ion mills, and FIBs tools, however we don't have enough people to handle the load and will not see an increase in headcount in the near future. I would appreciate any and all input on the following combinations of methods and equipment.
* wafering saw and FIB
vs.
* semi-automated polisher and ion mill
vs.
* precision cleaving and FIB
Thank you in advance for your opinions and accounts of your experiences with those approaches.
Regards,
Jerzy
****************************************************** Jerzy Gazda, Ph.D. Advanced Micro Devices Supervising Engineer 5204 E. Ben White Blvd. - MS 613 PCAL - AIM Section Austin, TX 78741 TEL: 1-800-538-8450, Ext. 51453 FAX: (512) 602-7470 jerzy.gazda-at-amd.com ******************************************************
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Does anyone have experience fixing and embedding fish embryos in plastics (epoxies or methacrylates) for serial sectioning? Advice, references and warnings are all appreciated!
Geoff -- ********************************************** Geoff McAuliffe, Ph.D. Neuroscience and Cell Biology Robert Wood Johnson Medical School 675 Hoes Lane, Piscataway, NJ 08854 voice: (732)-235-4583; fax: -4029 mcauliff-at-umdnj.edu **********************************************
I purchased "Via Voice" because I wanted to use it on a Mac and of course the choices for Mac were more limited. I also didn't want to spend a lot of money. For me, this seems to be a farely sophisticated program for a very reasonable price. It is, however, difficult to use if there is other noise in the room. I can only use it in a private office.
Bob Research Scientist U of Washington
On Tue, 17 Sep 2002, John J. Bozzola wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } I apologize is this is not strictly a microscopy question. A } microscopist colleague/friend of mine is interested in purchasing a } high quality speech recognition software. The individual is } handicapped and does not full use of their hands and would be using } the software for scientific writing (primarily describing microscopy } findings). Although I favor the Macintosh system (since they would } also use the computer for image processing and publishing), I am } looking for the best software to assist this individual. Any } recommendations would be appreciated. Many thanks. } } JB } } ############################################################## } John J. Bozzola, Ph.D., Director } I.M.A.G.E. (Integrated Microscopy & Graphics Expertise) } 750 Communications Drive - MC 4402 } Southern Illinois University } Carbondale, IL 62901 U.S.A. } Phone: 618-453-3730 } Fax: 618-453-2665 } Email: bozzola-at-siu.edu } Web: http://www.siu.edu/~image/ } ############################################################## } }
Can anyone suggest an independent service engineer who could perform a routine maintenance on our Philips EM 201 (we are located in New Haven, Connecticut)? The scope is currently down with a vacuum problem.
Please contact me offline if you have any leads!
Regards,
Stefan
°°°°°°°°°°°°°°°°°°°°°°°°°°°°°°°° Stefan Geimer MCDB Dept. Yale University P.O. Box 208103 New Haven, CT 06520-8103 U.S.A.
Dear all, Does anyone have any good electropolishing recipes for Co-Ni alloys? We have a Struers Tenupol. Suggestions for voltage and temperature would be good too.
Thanks in advance
-- Ian MacLaren Strukturforschung, Materialwissenschaft, TU-Darmstadt, Germany ian.maclaren-at-physics.org / http://homepages.tu-darmstadt.de/~maclaren/
I am looking for a reference that documents various anomalies associated with electroplating and electroless plating of metals such as gold, copper, nickel, zinc, etc., as seen through the SEM.
I took a tour through Amazon's bookshelves but didn't see anything that matched what I was looking for.
Greetings Dwight, I posted a very similar on the MSA Listserver about this time last year. The listserv archives can be searched using the interface at http://www.msa.microscopy.com/MicroscopyListserver/SearchMLArchive.html, however I can't seem to get the results I'm looking for using it--I posted a summary of the responses I received last year on 9/26. I managed to pull up the whole exchange in my Eudora archives, so I've appended the summary in the hope it provides you with the info you are after. I have been using spectroscopic grade MeOH dried with 4 angstrom molecular sieves in conjunction with cotton tipped swabs and filter paper. Usually a confident swab in one direction across the lens while simultaneously turning the shaft of the swab removes contamination. I use a new swab for every wipe, and the swab is dampened with only enough MeOH so that I can watch the trailing edge of the solvent rapidly evaporate behind the swab as I move it across the lens. Contamination should be trapped in the cotton tip of the swab--a similar process can be performed using strips of lens tissue dragged across the lens if you are afraid the swab might scratch the lens surface. I observe the whole operation with the objective placed under a dissecting microscope so that I can see what I'm doing, and whether it has been effective. The lens cleaning summary follows:
Greetings, I would like to thank all who offered their advise regarding the cleaning of objectives, and remedies for misused optics. I had included the suggestion of sonicating in acetone for comic relief (the rest of my friend's suggestion was that at least then I could put a hook through the hole where the lens used to be and use it as an ornament), however I do appreciate the concern which was expressed by many of you. Your suggestions have been very helpful and are much appreciated. I even learned how to make purple Sparkle glass cleaner clear (apparently the purple dye is photolabile). It appears that lens cleaning is a craft, the art of which is developed through trial and experience. There are many different approaches to the cleaning of objective lenses, however the underlying philosophies may be grouped under three major headings: 1.) physical interaction with the lens surface, 2.) the use of aqueous or water soluble cleaning solutions, and 3.) the dark art of organic solvents. An interesting non-solvent method I have come across is to fracture a piece of expanded polystyrene (packaging material) and to use the freshly exposed surface to clean the lens (press into the lens and rotate). This method was recommeded by Leitz (now Leica) in the past. Apparently the method is effective and will not scratch the lens. For light duty cleaning, various formulations of aqueous solvent/detergent mixtures seem to be popular. These cleaning solutions include Kodak lens cleaner, Windex, and Sparkle. Some people recommend cutting the concentration of these solutions with distilled water (50%). Sparkle seems to have somewhat of a cult following-it is alcohol and ammonia free-and it is what we have been using here for some time. In all cases, care must be taken to drag the contamination and grit away from the lens using lens tissue. Work from the inside of the lens out, and make sure not to smear contamination across areas which you have just cleaned (use the lens tissue to trap the contamination, not just move it around). The aqueous detergent methods seem to be safe for lens coatings. Oil objectives do not need to be cleaned with detergent each use-wiping the oil off with lens tissue should suffice as long as different formulations of immersion oil are not being used on the same objectives. Apparently, immersion oils from different sources can react to produce a sort of sludge which is then more difficult to remove. Also, old-fashioned natural immersion oils such as pine oil have a volatile component which will evaporate and leave a gummy residue behind. Inverted microscopes may benefit from the use of little "diapers" for the objective lenses which absorb excess oil and prevent it from leaking back into the objective. Preventative maintenence is the goal here. The use of organic solvents is not for the faint of heart, however some brave souls manage to use these methods without incident. The less fortunate tell tales of leaking lenses (a problem particularly on inverted scopes) and even lens components dropping out of the barrel of the objective. Attention to proper technique is important. High quality cotton tipped applicators are favored for cleaning objectives with strong solvents-some people make their own and some people purchase them. A common theme is to begin at the center of the lens and work outward, slowly rotating the cotton swab so as to pick up the contamination rather than drag it about the lens. Using a dry applicator or reusing any portion of the applicator can scratch the lens. The cement which holds the lens together is easily dissolved using some of these solvents, and so great care must be taken not to "drown" the lens in solvent. The applicator should be neither dry nor saturated with solvent. It is important not to touch the cotton and contaminate it with oil from one's fingers. In an alternative method, one gently and unidirectionally drags a single-use strip of lens paper dampened in one spot with the solvent across the lens. Favored solvents include: lighter fluid (apparently used by some service reps), anhydrous ether, a mixture of diethylether and benzene, spectroscopy grade chloroform, isopropanol, methanol and xylene. There are others, to be sure. A common final touch is to fog the lens using distilled water from one's breath, and polish with one unidirectional swipe of a high quality lens paper. I hope this summary helps those of you who have expressed interest in the subject of objective cleaning and once again I thank everyone for thier input. Best Regards, Karl G.
At 07:17 PM 9/17/2002 -0500, Dwight Arrieche (IIBCA)" (by way wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
_______________________________________________ Karl Garsha Light Microscopy Specialist Imaging Technology Group Beckman Institute for Advanced Science and Technology University of Illiniois at Urbana-Champaign 405 North Mathews Avenue Urbana, IL 61801 Room B650J Tel: (217) 244-6292 Fax: (217) 244-6219 www.itg.uiuc.edu
You could try a 50:50 mix of Windex (or any clear window-cleaning fluid) and distilled water. Use Kimwipes or cotton buds or cloth, never Kleenex, with many gentle wipes rather than a few vigorous ones, and be careful to dry the lens at the end. Hope this helps.
Lesley Weston.
on 17/09/2002 5:17 PM, Dwight Arrieche (IIBCA) (by way of MicroscopyListserver) at darriech-at-cumana.sucre.udo.edu.ve wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } } Dear List Servers } } I need some help for cleaning or removing oil from LM lenses. } What is the recommended method and solvents for this task? } } Thanks } } D. Arrieche } IIBCA-UDO } darriech-at-cumana.sucre.udo.edu.ve }
Has anyone experience with embedding whole human lung in paraffin or methacrylate, especially if the lung was previously air-dried while inflated? Thanks, Tom
Thomas Moninger (thomas-moninger-at-uiowa.edu) University of Iowa Central Microscopy Research Facility (www.uiowa.edu/~cemrf) View expressed are my own.
Richard, I would like to remind you that there will be a TEM symposium at next year's M&M meeting. If you want to write it up, that may be the perfect place.
-Scott
Scott D. Walck, Ph.D. PPG Industries, Inc. Glass Technology Center P. O. Box 11472 (letters) Guys Run Rd. (packages) Pittsburgh, PA 15238-0472
Walck-at-PPG.com
(412) 820-8651 (office) (412) 820-8515 (fax)
-----Original Message----- } From: Richard Beanland [mailto:richard.beanland-at-bookham.com] Sent: Wednesday, September 18, 2002 8:16 AM To: 'jerzy.gazda-at-amd.com' Cc: Microscopy-at-sparc5.microscopy.com
Hi Jerzy, we have a similar workload to you, but in III-V's (we have looked at 475 TEM samples since April 1). We have only 2 people (myself and one other) doing all the sample prep, TEM and report writing. Much of our work is straightforward thickness measurements and cross-sections, and we have no FIB.
Do you have a Gatan PIPS or similar low-angle ion mill, with the ability to mill from predominantly one direction? I've found a great way of making cross sections using this machine combined with precision(ish) cleaving, cutting out several stages from the 'standard' way of doing things. Typical InP cross sections take less than an hour to do; with the right kind of sample (i.e. not site specific in 2 dimensions) it is possible to stack them up and do up to 10 at a time. It's straightforward to hit features down to 20um in size, but if you want to keep the specimen you really have to do one at a time. (It's impossible to get several specific sites thin at the same time, meaning you have to look at the first region that becomes electron transparent, then destroy it while getting the next one thin, etc..) Si takes longer since it ion mills so much more slowly, but the few I've done still take less than 90 mins from getting the sample to looking at it in the TEM.
I've been thinking of writing this up and publishing it somewhere, since it has saved us a huge amount of time and effort. I'm sure that if you were working with Si all the time you'd be able to optimise the procedure still further. I'll try to get some words together describing the procedure, with pictures, if you like.
FIB is great for very specific sites (less than 10um or so, depending on the structure) and I do use one in a tame academic's lab every so often, but for fast cross sections with lots of thin area I can't beat 'standard' methods. However I appreciate that Si geometries are often several orders of magnitude smaller and more complex than III-Vs, and site specific samples are likely to be a much bigger proportion of your workload.
-----Original Message----- } From: "jerzy.gazda-at-amd.com"-at-sparc5.microscopy.com [mailto:"jerzy.gazda-at-amd.com"-at-sparc5.microscopy.com] Sent: 17 September 2002 23:09 To: Microscopy-at-sparc5.microscopy.com
Dear Listers,
We are forced to evaluate methods of improving efficiency of sample preparation in our TEM laboratory and would like to hear your opinions on the following semi-automated approaches. The lab processes nearly a 1000 TEM samples per year, mostly cross-sections of CMOS devices on Si wafers. We use manual polishing, dimpling, ion mills, and FIBs tools, however we don't have enough people to handle the load and will not see an increase in headcount in the near future. I would appreciate any and all input on the following combinations of methods and equipment.
* wafering saw and FIB
vs.
* semi-automated polisher and ion mill
vs.
* precision cleaving and FIB
Thank you in advance for your opinions and accounts of your experiences with those approaches.
Regards,
Jerzy
****************************************************** Jerzy Gazda, Ph.D. Advanced Micro Devices Supervising Engineer 5204 E. Ben White Blvd. - MS 613 PCAL - AIM Section Austin, TX 78741 TEL: 1-800-538-8450, Ext. 51453 FAX: (512) 602-7470 jerzy.gazda-at-amd.com ******************************************************
======================================================================= This e-mail is intended for the person it is addressed to only. The information contained in it may be confidential and/or protected by law. If you are not the intended recipient of this message, you must not make any use of this information, or copy or show it to any person. Please contact us immediately to tell us that you have received this e-mail, and return the original to us. Any use, forwarding, printing or copying of this message is strictly prohibited.
No part of this message can be considered a request for goods or services. ======================================================================= Any questions about Bookham's E-Mail service should be directed to postmaster-at-bookham.com.
I am curious. If you have an FIB, why don't you set up several sample areas to be milled overnight, come in a clean them up, and then use the pluck-out system? If you have multiple samples, you could cut them down or cleave them and mount them on a holder and then use the auto milling program.
-Scott
Scott D. Walck, Ph.D. PPG Industries, Inc. Glass Technology Center P. O. Box 11472 (letters) Guys Run Rd. (packages) Pittsburgh, PA 15238-0472
Walck-at-PPG.com
(412) 820-8651 (office) (412) 820-8515 (fax)
-----Original Message----- } From: "jerzy.gazda-at-amd.com"-at-sparc5.microscopy.com [mailto:"jerzy.gazda-at-amd.com"-at-sparc5.microscopy.com] Sent: Tuesday, September 17, 2002 6:09 PM To: Microscopy-at-sparc5.microscopy.com
Dear Listers,
We are forced to evaluate methods of improving efficiency of sample preparation in our TEM laboratory and would like to hear your opinions on the following semi-automated approaches. The lab processes nearly a 1000 TEM samples per year, mostly cross-sections of CMOS devices on Si wafers. We use manual polishing, dimpling, ion mills, and FIBs tools, however we don't have enough people to handle the load and will not see an increase in headcount in the near future. I would appreciate any and all input on the following combinations of methods and equipment.
* wafering saw and FIB
vs.
* semi-automated polisher and ion mill
vs.
* precision cleaving and FIB
Thank you in advance for your opinions and accounts of your experiences with those approaches.
Regards,
Jerzy
****************************************************** Jerzy Gazda, Ph.D. Advanced Micro Devices Supervising Engineer 5204 E. Ben White Blvd. - MS 613 PCAL - AIM Section Austin, TX 78741 TEL: 1-800-538-8450, Ext. 51453 FAX: (512) 602-7470 jerzy.gazda-at-amd.com ******************************************************
I have been working on phase imaging of high impact polystyrene (HIPS), a composite of polystyrene and polybutadiene rubber particles, with DI AFM TappingMode. I have tried different microtoming conditions to optimize the cutting and therefore the imaging from those specimens, but with limited success. I have also found cutting temperature (tried from 0 C to -80 C) is very important but same temperature results in different cutting qualities, primarily chatters and local compressions on polystyrene matrix, from different specimens. However, -40 C is good for any specimens of impact copolymer of propylene and ethylene.
Does anybody have any experiences, suggestions or comments? Many thanks in advance.
Jiang Liu, PhD Research and Technology Center ATOFINA Petrochemicals (281) 884-0529 Jiang.liu-at-atofina.com
_________________________________________________________________ Chat with friends online, try MSN Messenger: http://messenger.msn.com
Working in a clinical lab of a hospital we are under pressure to eliminate latex gloves in favor of nitrile and now vinyl. Does anyone have appropriate references to support any of these, none of these or some of these? Thanks in advance for your help. F. Maiers
Sharon, We have been using an EPSON Expression 1600. The film holders did not come in 3.5x4 but I use the holder for four - 4x5s and with 3 sides supported, all is well. The machine works well, the limitation is my lack of knowledge in working in Adobe to make the images look their best. Pat Connelly Univ. of Pennsylvania, Biology Dept.
You may want to try "The Electrodeposition Of Tin And Its Alloys" by Dr Manfred Jordan ISBN 3-87480-118-7 This is an excellent reference with lots of SEM pictures.
Robert Fowler Quality Assurance Technician (Failure Analysis) TDK Components USA, Inc. Multilayer Ceramic Capacitor Division 1 TDK Boulevard Peachtree City GA 30269-2051 Telephone: (770) 631-0410 Ext.315 Fax: (770) 487-1460 email: rfowler-at-tdktca.com www.tdk.com
"Oakley, Jeff" {oakleyj-at-rayov To: "MSA listserver" ac.com} {Microscopy-at-sparc5.microscopy.com} cc: 09/18/2002 Subject: book search / plating anomalies 11:37 AM
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I am looking for a reference that documents various anomalies associated with electroplating and electroless plating of metals such as gold, copper, nickel, zinc, etc., as seen through the SEM.
I took a tour through Amazon's bookshelves but didn't see anything that matched what I was looking for.
by asking for an independent service I did not want to imply that I ever was dissatisfied with the Fei/Philips service. In my lab in Germany we have a CM 10 which is serviced by Fei/Philips for over 10 years and they always did a great job and sometimes even more than that! Looking for an independent service for the 201 has more to do with the age of the instrument. I don´t know if Fei services instruments that old, but was in the process of contacting them and get this information.
Post doctoral position available at the University of New Orleans/ Advanced Materials Research Institute (AMRI)
Requirements : Background in Materials Sciences and experience in the operation of a TEM
Project : Li-ion batteries are used as power source in portable electronics and medical devices. After high cycle number the capacity of these batteries decreases which is partly due to structural instabilities of the cathode (LiCoO2). The study the crystal structure and lattice defects in LiCoO2 before and after electrochemical cycling is aimed at a better understanding of the failure mechanisms leading to the reduced performance.
Contact : Heike Gabrisch Assistant Professor of Chemistry Department of Chemistry/AMRI University of New Orleans New Orleans, LA 70148
I have a recipe I can share from Bernie Kestel which was used on our Model 550 Jet Polisher. I'm sure it won't translate exactly to your equipment, but it may be a good starting point. I hope it helps.
Material: Ni-10Co
Electrolyte: 10% HClO4 90% ethanol
Temperature: 0 degrees C
Jet Height: 3.9mm
Pump Speed: 2-4
Volts: 20
Current: 35 mA
Comments: After termination, rinse specimen immediately.
This is from an Argonne National Lab Publication (ANL-80-120) titled "Polishing Methods for Metallic and Ceramic Transmission Electron Micrscopy Specimens" by Bernie Kestel.
I don't know if it is available from Argonne anymore, but I can supply you with a copy of the booklet (about 60 pages) if you think it would be useful. It discusses many different jet polishing techniques although the majority of it is done with one of our Model 550 Jet Polishers.
Best regards-
David
DISCLAIMER: South Bay Technology produces equipment and supplies as described above and, therefore, has a vested interest in promoting their use.
-- David Henriks TEL: +1-949-492-2600 South Bay Technology, Inc. FAX: +1-949-492-1499 1120 Via Callejon San Clemente, CA 92673 USA e-mail: henriks-at-southbaytech.com
*** www.southbaytech.com ***
Ian MacLaren wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } Dear all, } Does anyone have any good electropolishing recipes for Co-Ni alloys? We } have a Struers Tenupol. Suggestions for voltage and temperature would } be good too. } } Thanks in advance } } -- } Ian MacLaren } Strukturforschung, Materialwissenschaft, TU-Darmstadt, Germany } ian.maclaren-at-physics.org / http://homepages.tu-darmstadt.de/~maclaren/
Hello Dwight, I compiled answers to your question from a previous inquiry a year or so ago. Let me know if it helps. I have pasted it in at the end of this message. Dean Abel Biological Sciences 138BB University of Iowa Iowa City IA 52242-1324
At 07:17 PM 9/17/2002 -0500, you wrote: ------------------------------------------------------------------------ The Microscopy ListServer -- Sponsor: The Microscopy Society of America
BEST SOLVENT FOR REMOVING IMMERSION OIL FROM OBJECTIVE LENS
I asked if xylene was the best solvent for cleaning immersion oil off a non-immersion objective. Here is the array of responses I received. The diversity may interest you.
1. We regularly use xylene with a cotton tipped applicator to clean our lenses and remove immersion oil. This was recommended to us by the supplier of our lenses and microscopes for a number of reasons. The primary reason is that xylene effectively 'cuts' the oil, without damaging the lens. Acetone will affect the lens coating, and isopropyl alcohol only rinses the oil without effectively removing it.
2. Use alcohol on lens paper. Never use xylene or toluene; these solvents can dissolve the cement used to seat the various lens elements.
3. I would recommend Sparkle Glass Cleaner. I only use solvents as a very last resort. The cements are soluble in most solvents. With intractable grime, I use a cotton tipped applicator moistened with either xylenes or toluene and shake all excess off. The tip must be moist, not wet or dry, and make single passes until the grime come off. Use only enough solvent on the applicator to dampen the surface, not enough to wet.
4. For day-to-day cleaning of lenses, including oil on the 40X, invert an ocular and examine the surface for cleanliness. If it is clean, don't clean it. Dust off any loose debris. Check the lens again. Moisten a cotton tipped applicator in Sparkle and wipe the lens once with a rolling action to present a new surface and lift off any grit. Discard. Take a dry applicator and remove the film. Check the lens with an inverted ocular to see if it is clean. Do no more than is necessary.
5. The care instructions for my immersion oil suggest cleaning with a soft cloth or lens tissue (no Kimwipes) moistened with ether/alcohol (7:3) or xylenes. My microscope manuals recommend removing fingerprints using alcohol
6. We use 70 % isopropanol to clean immersion oil off of our lenses.
7. Cleaning with xylene is a little drastic. If the lens eventually gets xylene in behind the cement it could do some damage and you would have to send it in for repair. I use Kodak lens cleaner and some lens cleaning tissues (not Kimwipes) to get the oil off, constantly checking under a dissecting scope to make sure that it is all removed. This works well on some expensive lens that we have here.
8. We use Green Soap from the pharmacy. It works best with ultra pure water.
9. Alcohol is usually safer than xylene, but safer still is diluted detergent, such as "Joy" or similar, followed by water. Use alcohol only if that doesn't work. Fumes from xylene, toluene, etc. are best avoided.
10. Back in the old days, toluene was a recommended solvent for cleaning lenses of immersion oil. These days we wipe off excess oil with lens tissue and then clean the lens with Kodak lens cleaner solution.
11. The best way to clean immersion oil from a lens is to use lighter fluid. First remove as much oil from the lens with lens paper. Be gentle; don't rub. Then dip a cotton swab in the lighter fluid and lightly wipe it across the lens. All the oil will be removed and it will evaporate very quickly without leaving a residue or streaks. Xylene is not recommended as it can dissolve the adhesives holding the lens in place.
Hi Microscopy Folks, I am trying to find a commercial or perhaps university lab which will allow us to so some SEM cathodoluminescence measurements on carbon field emitters. Any pointers? Thanks, Greg M.
Microscopists, I have a run of Journal of Cell Biology from 1987 through 2001 that I would like to give away. Our library doesn't want them. Anyone out there interested? Or know of a connection to libraries somewhere that might be interested?
Jeff, I only have experience in imaging electroless copper by TEM. TEM shows small bubbles in the metal. I don't remember the details as this was some time ago. I believe they are produced by Hydrogen, which tends to make the metals more brittle.
Don Werder
Oakley, Jeff wrote:
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You may want to check publications from ASM international (www.asminternational.org). Start with Volume 5 (10th edition) of the Metals Handbooks-Surface Engineering. Volume 11 deals with Failure Analysis and Prevention and may have some examples. Good Luck.
Joseph
Joseph M. Oparowski Materials Science Research - Consulting and Failure Analysis Bose Corporation Joseph_Oparowski-at-bose.com The Mountain, M/S 415 Phone: (508) 766-1371 Framingham, MA 01701-9168 Fax: (508) 766-1313
-----Original Message----- } From: Oakley, Jeff [mailto:oakleyj-at-rayovac.com] Sent: Wednesday, September 18, 2002 11:38 AM To: MSA listserver
I am looking for a reference that documents various anomalies associated with electroplating and electroless plating of metals such as gold, copper, nickel, zinc, etc., as seen through the SEM.
I took a tour through Amazon's bookshelves but didn't see anything that matched what I was looking for.
You might want to contact Dr. Fred Hossler at hossler-at-ETSU.Edu. He is very helpful in these matters.
JD Arnott
Ladd Research 83 Holly Court Williston, VT 05495
On-line Catalog: http://www.laddresearch.com
tel: 1-802-658-4961(anywhere) or 1-800-451-3406(US) fax: 1-802-660-8859 e-mail: sales-at-laddresearch.com ----- Original Message ----- } From: "Tom Moninger" {thomas-moninger-at-uiowa.edu} To: {Microscopy-at-sparc5.microscopy.com} Sent: Wednesday, September 18, 2002 1:12 PM
Hi Folks I am curious if any of you using HF are utilizing the hf antidote gel. If you are where can I find some in US. Thank You
Robert Fowler Quality Assurance Technician (Failure Analysis) TDK Components USA, Inc. Multilayer Ceramic Capacitor Division 1 TDK Boulevard Peachtree City GA 30269-2051 Telephone: (770) 631-0410 Ext.315 Fax: (770) 487-1460 email: rfowler-at-tdktca.com www.tdk.com
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Listers, We, being non-material people, need some help with a material sample. The sample is a high impact polystyrene (HIPS) that contains butadiene rubber moieties. We need to be able to identify the location of these rubber moieties and understand that they will stain upon exposure to osmium. Does anyone have any experience with this type of sample. Would it be advisable to stain by floating thin sections (on grids) on liquid osmium or by using osmium vapors? What type of grids would be most desirable to minimize corrosion by the osmium?
Also, we have a diamond knife made by Diatech in Tennessee. I need to contact them to obtain information about this knife. Does anyone have a phone number or other contact information?
Debby
Debby Sherman, Manager Phone: 765-494-6666 Life Science Microscopy Facility FAX: 765-494-5896 Purdue University E-mail: dsherman-at-purdue.edu S-052 Whistler Building West Lafayette, IN 47907
} Hi Folks I am curious if any of you using HF are utilizing the hf antidote gel. If you are where can I find some in US. Thank You } } Robert Fowler } Quality Assurance Technician (Failure Analysis) } TDK Components USA, Inc. } Multilayer Ceramic Capacitor Division } 1 TDK Boulevard } Peachtree City GA 30269-2051 } Telephone: (770) 631-0410 Ext.315 } Fax: (770) 487-1460 } email: rfowler-at-tdktca.com } www.tdk.com }
One of our folks in my dept. worked at Ohio State in the group that used cathodeluminescence.
The contact he gave me at Ohio State is below.
Regards,
Peter Tomic Anadigics, Inc.
Professor Len Brillson Department of Electrical Engineering
-----Original Message----- } From: Greg Mulhollan [mailto:mulhollan-at-extremedevices.com] Sent: Wednesday, September 18, 2002 6:40 PM To: Microscopy-at-sparc5.microscopy.com
Hi Microscopy Folks, I am trying to find a commercial or perhaps university lab which will allow us to so some SEM cathodoluminescence measurements on carbon field emitters. Any pointers? Thanks, Greg M.
Hello listers, The University of New Hamphsire has a Hitachi H600 100 kV STEM with an H-6010 scanning system (working), an Oxford thin window EDS (working) and a PGT IMIX-PC system that we are in the process of replacing. The microscope was installed in 1986 and is not operational due to a high voltage buffer problem (we think). Also, the PGT Sun system needs a new hard drive (we think). The microscope has 2 sets of 30 plate film cassettes and boxes with vacuum film desiccator. We will be dismantling the scope soon. Interested parties looking for microscope parts, or interested in getting this one to work, please contact me with inquiries/offers off-line. It will be the donee's responsibility to come and take the microscope or pay removal, shipping and handling charges. I am open to discuss any offers. I will also post details on Nestor's surplus equipment list at the MSA website.
Thanks!
Dr. Jeff Simpson Electron Microscope Facility University Instrumentation Center University of New Hampshire Kendall Hall Durham, NH 03824 603-862-2457 jeff.simpson-at-unh.edu
Visit us at http://www.unh.edu/instrumentation-center/about.html
Listers, I am looking for a very fine grained film to use for capture of SEM images. We want to use this film in place of the Polaroid Type 55P/N film. Kodak recommends the Tmax 100 4x5 sheet film. I would appreciate other recommendations or confirmation that this would be the film of choice.
Thanks, Debby
Debby Sherman, Manager Phone: 765-494-6666 Life Science Microscopy Facility FAX: 765-494-5896 Purdue University E-mail: dsherman-at-purdue.edu S-052 Whistler Building West Lafayette, IN 47907
Debbie, There is some literature suggesting that ruthenium tetroxide is better than osmium for this kind of thing. There is a paper by Trent, Scheinbeim, and Couchaman 1983 Macromols 16: 589-598 that is very informative. My understanding is that it is usual to vapor stain this kind of sample. Hope this helps, Tobias } } } } Listers, } We, being non-material people, need some help with a material sample. } The sample is a high impact polystyrene (HIPS) that contains butadiene } rubber moieties. We need to be able to identify the location of these } rubber moieties and understand that they will stain upon exposure to osmium. } Does anyone have any experience with this type of sample. Would it be } advisable to stain by floating thin sections (on grids) on liquid osmium or } by using osmium vapors? What type of grids would be most desirable to } minimize corrosion by the osmium? } } Also, we have a diamond knife made by Diatech in Tennessee. I need to } contact them to obtain information about this knife. Does anyone have a } phone number or other contact information? } } Debby } } Debby Sherman, Manager Phone: 765-494-6666 } Life Science Microscopy Facility FAX: 765-494-5896 } Purdue University E-mail: dsherman-at-purdue.edu } S-052 Whistler Building } West Lafayette, IN 47907
Opening for an experienced EM tech. at the Univ. of Connecticut Health Center. Prefer candidate with clinical experience. Details available online at http://employ.uchc.edu/
Sorry if this is a duplicate, but the first time didn't seem to go through.
I have a HT tank for a Philips 300 which I have no use for. The part number is 4022 185 00651. It is already crated. I do not know if it is in working order. The crate has a RMA number on it, but I don't know it was fixed and returned or if it was never sent in for repairs.
Available to anyone who will cover shipping.
If I don't hear from any interested parties by the end of next week, I will pursue scrapping it.
Tom -- Thomas M. Murray Phone: (206)543-2836 Electron Microscopy Center Manager Fax: (206)543-3100 Materials Science & Engineering email: murraytm-at-u.washington.edu Roberts Hall 130 University of Washington Seattle, WA 98195
I would certainly consider Kodak Tech Pan 4415. Speed is dependent on development but will be slower than T-Max, around 25-32 and grain structure is very fine.
Rick A. Harris, Director Microscopy and Imaging Facility Section of Molecular and Cellular Biology 1241 Life Sciences Addition University of California Davis, CA 530 752 2914 http://katie.ucdavis.edu raharris-at-ucdavis.edu
} Listers, } I am looking for a very fine grained film to use for capture of SEM } images. We want to use this film in place of the Polaroid Type 55P/N film. } Kodak recommends the Tmax 100 4x5 sheet film. } I would appreciate other recommendations or confirmation that this would } be the film of choice. } } Thanks, } Debby } } Debby Sherman, Manager Phone: 765-494-6666 } Life Science Microscopy Facility FAX: 765-494-5896 } Purdue University E-mail: dsherman-at-purdue.edu } S-052 Whistler Building } West Lafayette, IN 47907
Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (HWHAMILT-at-UTMB.EDU) from http://www.msa.microscopy.com/Ask-A-Microscopist.html on Thursday, September 19, 2002 at 15:24:08 ---------------------------------------------------------------------------
Email: HWHAMILT-at-UTMB.EDU Name: Dub Hamilton
Organization: Utmb Galveston
Education: Graduate College
Location: galveston Texas
Question: I am interested in purchasing a microscope for 'serious hobby use'. A number are available at about $500 with a 1.25 adjustable abbe condensers.(looking at Accu-scopy a3025 and LW Scientific Observer IV) Questions: 1. Is this about right for me? 2. Is Kohler illumination possible with this condenser or is something eles required? 3.Is achromatic objectives ok for my purpose?
The method we use is to stain in Os vapour for 30 min to an hour on ultrathin sections. We normally use copper grids without any problems.
Put a couple of drops of 2% stock Os solution in a jar, position the grids above the liquid (we use an old flexible plastic grid holder) and leave capped in fumehood for the time.
Leave the jar open to air out after removal of Os at least overnight before discarding the jar and leave the grids open to air for awhile before putting in microscope to get rid of Os smell.
--
Ian Kaplin
Electron Microscope Unit Madsen Bldg F09 The University of Sydney NSW 2006 Australia
there is a product called Reachout which was designed forthis. I used it for a person totally disabled back in 1998.. he had an eyeball controlled keyboard and could use windows nt very well with it from his always "on the bak possition. he was paralyzed from his neck down.21 years old at time. you might search fo it I believe the people that made it were in Florida. if you need more help let me know.
sterling
On Tue, 17 Sep 2002, John J. Bozzola wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } I apologize is this is not strictly a microscopy question. A } microscopist colleague/friend of mine is interested in purchasing a } high quality speech recognition software. The individual is } handicapped and does not full use of their hands and would be using } the software for scientific writing (primarily describing microscopy } findings). Although I favor the Macintosh system (since they would } also use the computer for image processing and publishing), I am } looking for the best software to assist this individual. Any } recommendations would be appreciated. Many thanks. } } JB } } ############################################################## } John J. Bozzola, Ph.D., Director } I.M.A.G.E. (Integrated Microscopy & Graphics Expertise) } 750 Communications Drive - MC 4402 } Southern Illinois University } Carbondale, IL 62901 U.S.A. } Phone: 618-453-3730 } Fax: 618-453-2665 } Email: bozzola-at-siu.edu } Web: http://www.siu.edu/~image/ } ############################################################## }
Dear colleagues, C2 apertures in our CM12 are heavily contaminated. Does anybody could suggest how to clean them? Heating in molybdenum boat does not work. Thanks for any responses. O. Benada
+-----------------------------------+ Oldrich Benada Acad. Sci. CR Institute of Microbiology Laboratory of electron microscopy Videnska 1083 CZ - 142 20 Prague 4 - Krc Czech Republic +------------------------------------+ Phone: +420-2-41062399 Fax: +420-2-41062347 WEB: http://www.biomed.cas.cz/mbu/lem113/lem.htm
Debby I have used Kodak TMax 100 in 35mm and 120 (6x7cm) formats for many years and can thoroughly recommend it. In 6x7 cm images the film can record all of the data available from the SEM record monitor. Images are suitable for enlargement to at least 16x20", often 20x30" and at these mags film grain is much less important than image noise. I doubt if you would gain very much by using 5"x4", and the negatives would be much more trouble to process. However, there is significant loss of image quality when 35mm format is used. This may be unimportant for images of the size required in scientific publications, but degrades the quality of exhibition images. Chris
} Debby, } } I would certainly consider Kodak Tech Pan 4415. Speed is dependent on } development but will be slower than T-Max, around 25-32 and grain structure } is very fine. } } Rick A. Harris, Director } Microscopy and Imaging Facility } Section of Molecular and Cellular Biology } 1241 Life Sciences Addition } University of California } Davis, CA } 530 752 2914 } http://katie.ucdavis.edu } raharris-at-ucdavis.edu } } } } } } Listers, } } I am looking for a very fine grained film to use for capture of SEM } } images. We want to use this film in place of the Polaroid Type 55P/N film. } } Kodak recommends the Tmax 100 4x5 sheet film. } } I would appreciate other recommendations or confirmation that this would } } be the film of choice. } } } } Thanks, } } Debby } } } } Debby Sherman, Manager Phone: 765-494-6666 } } Life Science Microscopy Facility FAX: 765-494-5896 } } Purdue University E-mail: dsherman-at-purdue.edu } } S-052 Whistler Building } } West Lafayette, IN 47907 } }
Dear all, We are interested in purchasing a heating/tensile stage for our Phillips CM20 (Supertwin lens). We are intending to use this for studying deformation in thin films.
I would appreciate information and approximate prices from manufacturers.
I would also appreciate comments from users of such stages.
Thanks in advance
-- Ian MacLaren Strukturforschung, Materialwissenschaft, TU-Darmstadt, Germany ian.maclaren-at-physics.org / http://homepages.tu-darmstadt.de/~maclaren/
Here at Liverpool we have a VG HB 601 UX, which has developed a major fault within the way the probe is scanned. However, before the scanning fault developed, there were other intermittent faults and I feel that all these faults are connected. The first intermittent fault was an error message informing;
18:09:42 L9 Column Crate Interface Reset followed by 18:09:42 L9 Column Crate Interface 18:09:42 L9 Column Crate Interface +15V Failure This failure resulted in the stage translates not working. By rebooting both computers the fault would be cleared, this fault would happen once a week and then it progressed to once a day.
After rebooting sometimes the scanning would not be correct, i.e. instead of an image appearing we would just get parallel lines or the image of the VOA would be twisted and distorted. The faults have now progressed to a point of not being able to form an image at all in image mode, in Lo Mag Mode the image sometimes forms, however we can see it flick on and off without touching the console. In diffraction mode, sometimes we can see the objective aperture but usually no image of the ADF detector We have now lost all power to the middle and right hand side of the control panel and the console will not boot up anymore.
All help and ideas on where to start in rectifying these faults would be greatly welcome.
Adam
Please could all replies be to my e-mail address: ajp5-at-liv.ac.uk
-- Dr Adam Papworth, Senior Experimental Officer, Department of Engineering, The University of Liverpool, Liverpool, L69 3GH, UK.
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Dia-Tech Corporation 6408 Clinton Highway, Powell, TN 37849 (865) 938-2720
Robert Fowler Quality Assurance Technician (Failure Analysis) TDK Components USA, Inc. Multilayer Ceramic Capacitor Division 1 TDK Boulevard Peachtree City GA 30269-2051 Telephone: (770) 631-0410 Ext.315 Fax: (770) 487-1460 email: rfowler-at-tdktca.com www.tdk.com
Debby Sherman {dsherman-at-purd To: "message to: MSA list" ue.edu} {microscopy-at-sparc5.microscopy.com} cc: 09/19/2002 Subject: OS staining of rubber 01:01 PM
------------------------------------------------------------------------ The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Listers, We, being non-material people, need some help with a material sample. The sample is a high impact polystyrene (HIPS) that contains butadiene rubber moieties. We need to be able to identify the location of these rubber moieties and understand that they will stain upon exposure to osmium. Does anyone have any experience with this type of sample. Would it be advisable to stain by floating thin sections (on grids) on liquid osmium or by using osmium vapors? What type of grids would be most desirable to minimize corrosion by the osmium?
Also, we have a diamond knife made by Diatech in Tennessee. I need to contact them to obtain information about this knife. Does anyone have a phone number or other contact information?
Debby
Debby Sherman, Manager Phone: 765-494-6666 Life Science Microscopy Facility FAX: 765-494-5896 Purdue University E-mail: dsherman-at-purdue.edu S-052 Whistler Building West Lafayette, IN 47907
Plasma Cleaning is another solution which I have used on Condensor Apertures. Make sure you use the most reactive species possible... i.e. an Oxygen Rich Plasma.
If they are badly contaminated you may have to go to the high power Plasma Ashing regime.
However, if they are very heavily contaminated even that may not work since some residue may remain. In this case you will just have to replace them.
Disclaimer: My Employer ANL holds the Patent on Plasma Cleaning Technology for application to Electron Microscopy Specimens & In-situ Microscope applications. There are also commerical organizations which may be able to help you such as SPI, XEI, South Bay Tech and Fischione, all of whom are licensee's of the ANL Patent. Links to their respective WWW pages are on the WWW page below.
Check the 10/20 volt power supplies in the electronics racks. The symptoms you describe I have seen many times.
Look both at the fuses as well as the thermal sensors on each of the power supplies. Both of which are easily checked by measuring the resistance with an Ohm meter. Both of which have failed on my system at various times. I would tend to suspect the thermal sensor.
These units are located on my system (603Z) on the back of the Electronic Power Supply Rack, underneath the Objective Power Supply, on the 601 they might be elsewhere.
You can tell immediately if you have power to these units by looking for the "red" LED's on each of the units. They should be lit. If off, then power down the machine and pull the suspect unit and start checking each one. Start with the higher voltage supplies (20V) since they also supply power to a few of the lower voltage (10V) supplies.
Cheers....
Nestor Your Friendly Neighborhood SysOp.
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I have always felt that Polaroid P/N 55 was a very good choice for SEM image capture. While the positive print is nothing to write home about, the negative is of very high quality (in terms of sharpness, line to line resolution, and so on - granted it is rather low contrast). When printed on the old grade 4 Ilfobrom paper it gave excellent prints. I am assuming you are using fresh film, of course. A number of years ago I experimented with switching from Type 55 to conventional film, but my users wouldn't use it, and in the end I gave up on it myself. The fiddle of loading film holders and developing and printing wasn't worth the cost saving to most users. In the meantime they had working copies of all their images in the Polaroid positives. Not only that, but the conventional process required MUCH more support from me and my staff (how many of today's students knows the first thing about conventional B&W photography?)
The resolution and graininess of large format films for SEM images is usually quite unimportant, because the limiting factor in the image quality is the screen of the CRT. Even a relatively coarse-grain film like the old Kodak Tri-X can resolve better than 50 lines/mm (fine-grain films can resolve over 300 lines/mm). To generate this amount of information, on a 10cm^2 image, would require 10,000x10,000 pixels. I don't know of a CRT that can resolve that!
Of course, other labs' priorities may not be that same as mine, and there may be excellent reasons to switch from Polaroid, but my choice was to not follow that route.
Tony.
At 02:55 PM 9/19/2002 -0500, Debby Sherman wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
** Anthony J. Garratt-Reed ** MIT Room # 13-1027 ** 77 Massachusetts Avenue ** Cambridge, MA 02139-4307 ** USA ** ** Phone: (+) 1-617-253-4622 ** Fax: (+) 1-617-258-6478 **
We routinely use concentrated HF in our lab. and keep calcium gluconate gel for first treatment. However, be aware that it is a first treatment after a water rinse and you should get to a hospital ASAP or risk losing some tissue or worse.
Here are the details:
Manufactured by:
Calium Gluconate Gel
Calgonate Corp. Rhode Island, USA
Distributed by:
Pharmascience Inc. Montreal, Canada
You may call 1-800-363-8805 for info.
Regards,
Peter Tomic Anadigics, Inc. Warren, New Jersey The United States of America
-----Original Message----- } From: Kai Lorcharoensery [mailto:kai-at-lehigh.edu] Sent: Thursday, September 19, 2002 2:36 PM To: microscopy-at-sparc5.microscopy.com
The gel is calcium gluconate. You can buy a few tubes from Fisher (HF antidote gel) or Pharmascience.
Kai Lorcharoensery Materials Science & Engineering Lehigh University 5 E. Packer Ave. Bethlehem, PA 18015
} Hi Folks I am curious if any of you using HF are utilizing the hf antidote gel. If you are where can I find some in US. Thank You } } Robert Fowler } Quality Assurance Technician (Failure Analysis) } TDK Components USA, Inc. } Multilayer Ceramic Capacitor Division } 1 TDK Boulevard } Peachtree City GA 30269-2051 } Telephone: (770) 631-0410 Ext.315 } Fax: (770) 487-1460 } email: rfowler-at-tdktca.com } www.tdk.com }
Mick Thomas was inquiring about SF6 safety. Ah, that brings back such fond memories. Back in my days at SLAC, we were using SF6 as the high voltage insulating gas for our polarized electron gun. We spent a good deal of time determining risk levels since the gun operated in a relatively unventilated underground tunnel separated from the other sections of the accelerator by large doors. Here are a few of the items we determined: 1. SF6 is an asphyxiant and not a poison. In its pure form it is pretty unreactive. 2. SF6 is quite heavy and will immediately sink to floor level if there are in intervening flow barriers. You can consider SF6 as being trapped somewhere if you think of the analogous amount of water being poured from or contained in a vessel. In other words, if you have a big vessel filled with SF6 and open the top, it will retain a good deal of the SF6 for quite some time and still contain very little oxygen! 3. Filling our gun injector room with one complete large bottle of SF6 resulted in only about one inch of an oxygen depleted layer at floor level. 4. SF6 after having been in the presence of high voltage arcing, will break down forming some pretty nasty fluorimers, but generally at low concentrations.
In summary: SF6, due to its weight and (usual) inert qualities presents little risk, except if it is trapped in something or is broken down to its sub-components. Hope that helps.
Greg M.
} Fellow microscopists, } } I would be very grateful if someone could offer me advice on how to } ensure that a microscopy room is set up to safely handle a leak of } SF6. } } Thank you very much for your time and help. } } Sincerely, } } Mick } } ------------------------------------------------- } Mick Thomas } UHV-STEM Laboratory } E-1 Clark Hall } Cornell University } Ithaca, NY 14853 }
} } Hi Folks I am curious if any of you using HF are utilizing the hf antidote } gel. If you are where can I find some in US. Thank You } } Robert Fowler ************************ I buy my HF from Aldrich Chemicals. Lee -- Leona Cohen-Gould, M.S. Sr. Staff Associate Director, Electron Microscopy Core Facility Manager, Optical Microscopy Core Facility Joan & Sanford I. Weill Medical College of Cornell University voice (212)746-6146 fax (212)746-8175
Listers, I arrived at work today to find a number of responses to my earlier post asking about film for SEM. I have listed them below without reference to sender. I also had a number of responses asking why I wanted to use film for SEM. This is a good question since for 99% of our SEM work we do capture digital images and they are adequate for most purposes. However, I guess I am still from the old school. I still find film better than digital if you want to enlarge images. In this particular case, we are hoping to purchase a high resolution FESEM. A goodly percentage (not all) of the samples will be very small...things like viruses, liposomes, and various nanoparticles with sizes ranging from 10nm up. Although the newest models of FESEM can resolve these structures, even though we will also have to deal with cryo conditions as most samples will be hydrated, there is still the problem of "empty magnification" when taking the original image. This limit to the useful magnification when we originally capture the image is the potential problem. In many cases we envision that we may need to substantially enlarge single particles to illustrate finer features to our audience. In this case, using very fine grained film will give us more opportunity to increase size without concern for pixelization or without having a computer decide how to insert smaller pixels (as would happen if we just punch in a higher resolution figure and let the computer interpret). In fact, it surprises me that for a relatively small sum when considering the cost of the entire instrument package, many people do not choose to have the option of using film when purchasing a new high resolution instrument. You may never use it but you may well wish to have the option sometime down the road.
Again, thanks to all who responded. I may get a few more responses as the day goes on but wanted to get this off before it gets buried in my in box. As to final choice of film....I plan to try a number of the suggested ones and see what fits our needs.
Debby
==============
Tmax is a bit on the contrasty side. For wider range, I prefer Ilford FP4+ (rated ISO125, shoot at ISO 100).
This film comes in sheets and rolls (120/220). You can use cut film holders for 4x5 or use a 6x7cm or 6x9cm roll back for use with the roll film. Horseman or Wista are the best brands of roll film backs. These slide into the Graflok back where the Polaroid back was. Remove the ground glass clam shell affair by pressing the two chrome latches and slide the ground glass off the photo unit.
Roll film approach is cheap and very easy to use. Not the same size as 4x5 but you have the option.
==========
I would certainly consider Kodak Tech Pan 4415. Speed is dependent on development but will be slower than T-Max, around 25-32 and grain structure is very fine.
========== I have used Tech pan 120 roll film in the past and found it to be a very fine grained film. Of course you don't get positives untill you develop it, although you wouldn't get positives with the Tmax 100 sheet film either.
============= T-max 100 is excellent film which I have used in both 35mm as well as 4"x5" formats and have been extremely satisfied with the grain size. I'm not sure if it comes in quick load sheets which would look just like the polaroid type 55 film and also uses the 545 holder but it probably does. Otherwise just get a few film holders. They are not going to be around much longer, although people have been saying this for years. ===========
I have used Kodak TMax 100 in 35mm and 120 (6x7cm) formats for many years and can thoroughly recommend it. In 6x7 cm images the film can record all of the data available from the SEM record monitor. Images are suitable for enlargement to at least 16x20", often 20x30" and at these mags film grain is much less important than image noise. I doubt if you would gain very much by using 5"x4", and the negatives would be much more trouble to process. However, there is significant loss of image quality when 35mm format is used. This may be unimportant for images of the size required in scientific publications, but degrades the quality of exhibition images. =============
I used Agfa APX 100 in 120 rollfilm for SEM images. It exist too in 4x5". So fine as the T-max and much cheapper. For normal use, I develop it with Rodinal 1+25. For fine grain use, it's better to use Attomal-FF
=============
Debby Sherman, Manager Phone: 765-494-6666 Life Science Microscopy Facility FAX: 765-494-5896 Purdue University E-mail: dsherman-at-purdue.edu S-052 Whistler Building West Lafayette, IN 47907
Robert Fowler wrote: =========================================== Maybe this is the location you want?
Dia-Tech Corporation 6408 Clinton Highway, Powell, TN 37849 (865) 938-2720 =========================================== This is a non-working number and so far as I know, they are no longer in busienss.
However, there are several firms that would be able to resharpen diamond knives made by Dia-Tech including SPI, MicroStar, DDK, Drukker and others.
Chuck
PS: Remember that we are striving to be 100% paperless, therefore there are no paper copies kept of this correspondence. Please be sure to always reply by way of "reply" on your software so that the entire string of correspondence can be kept in one place. ============================================
Charles A. Garber, Ph. D. Ph: 1-610-436-5400 President 1-800-2424-SPI SPI SUPPLIES FAX: 1-610-436-5755 PO BOX 656 e-mail:cgarber-at-2spi.com West Chester, PA 19381-0656 USA Cust.Service: spi2spi-at-2spi.com
Look for us! ######################## WWW: http://www.2spi.com ######################## ============================================
Debby, We routinely examine HIPS material in the TEM. Our method is to stain the trimmed and faced sample block in liquid Osmium solution (2% aq) before sectioning. Just place the block in a sealed bottle of solution, only enough to cover is needed, and leave in your hood overnight. Remove in the morning into a small bottle of tap water in the hood for 5 minutes or so, then set the block out in the hood to air dry for a half hour or so. The block should be much darker. Room temperature section as you normally would. Make a careful approach, because the stain will only penetrate for on the order of 10 sections -at- 100nm. 70nm to 90nm sections look very good. HIPS stains very well with this method. Some HIPS samples will warp, making approach more difficult, but usually only to an annoying rather than catastrophic degree. If you have problems, please contact me off-list about recalcitrant samples. Sincerely, Matt
Matthew K. Stephenson Analytical Associate Impact Analytical 1910 West Saint Andrews Road Midland, MI 48640 (989) 832-5555 X506 stephenson-at-impactanalytical.com
-----Original Message----- } From: Debby Sherman [mailto:dsherman-at-purdue.edu] Sent: Thursday, September 19, 2002 1:02 PM To: message to: MSA list
Listers, We, being non-material people, need some help with a material sample. The sample is a high impact polystyrene (HIPS) that contains butadiene rubber moieties. We need to be able to identify the location of these rubber moieties and understand that they will stain upon exposure to osmium. Does anyone have any experience with this type of sample. Would it be advisable to stain by floating thin sections (on grids) on liquid osmium or by using osmium vapors? What type of grids would be most desirable to minimize corrosion by the osmium?
Also, we have a diamond knife made by Diatech in Tennessee. I need to contact them to obtain information about this knife. Does anyone have a phone number or other contact information?
Debby
Debby Sherman, Manager Phone: 765-494-6666 Life Science Microscopy Facility FAX: 765-494-5896 Purdue University E-mail: dsherman-at-purdue.edu S-052 Whistler Building West Lafayette, IN 47907
Hello, I am a beginner in the EDX field. Is there any free software which could allow to list the possible energie interferences for a given matrix ? thanks and regards
Claude GRATTEPAIN
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I just cleaned my condenser aperature using metal polish on a cotton swab. The same I use to clean the wehnelt. It took care of the very heavy contamination. I sonicated in acetone two changes for 5 min. each and its now working fine. You cannot do this with thin foil aperatures (ie. objective aps.)
Where I work, I have the luxury of a metallographic lab available. To clean apertures, I simply use diamond polishing compound and napped cloth. I use the tip of my finger to move the aperture in the diamond compound around on the cloth until the contaminants are gone. It usually takes just a few seconds. Follow up with ultrasonic cleaning and rinsing.
I believe this method is far superior and easier than baking in removing contaminants. Keep in mind there is always the risk of catching a corner and folding the aperture, rendering it useless, which hasn't happened to me yet.
Stu Smalinskas SKF NATC Plymouth, Michigan
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As described in the MSA Bylaws, article 4, section 3, paragraph e, I wish to apply for emeritus membership in MSA. I have been a member since 1966, have been President of the Local Affiliated Society in Iowa and will retire from employment at Iowa State University on December 31, 2002. Please contact me if you need additional information.
I don't know about specifics for the Mac, but have some Wintel specifics and general information to offer:
The two "leading" packages for the PC are IBM ViaVoice and Dragon NaturallySpeaking (made by ScanSoft).
Both have a line of products that very in level of sophistication. They also both offer specialized versions for specific industries, including Medical and Legal. I'm not sure if they have "scientific" modules or not. The modules basically add specialized vocabulary.
There is a matrix of capabilities that are common to most voice recognition software. One side of the matrix is the "training side", the other is the "function side".
On the function side, there are basically two modes: Command mode, and dictate mode. Dictate mode allows dictation (e.g. microscope observations) into an application. Most of the PC based system can integrate with the common software, as well as just provide "keyboard" mimicking into any application that accepts text. The integration with something like Word provides the ability to handle formatting as your dictating. The command mode provides access to the Windows interface, and control of applications and the windows environment. Most dictating capable products include command mode, but you can find "command mode" only navigators (probably not appropriate in this case).
On the training axis, there is a continuum. In a perfect world, a voice recognition system could allow anyone to walk up and start using it with 100% accuracy. The problem here is that we don't all have a monotone voice with perfect Midwest (pick your geographic area) diction. Not to mention foreign languages and industry specific "jargon" and terminology. There are programs that do try and do this, and they are "speaker independent" systems. While these systems are getting better as processing power and programming techniques get better and faster, they tend not to be as robust and accurate as systems that provide some level of training.
The speaker dependent systems will require varying degrees of training before the system will work. This generally involved reading a paragraph or two. From this sample paragraph(s), the system builds a profile of how to recognize the voice. The more training the more accurate (in general). The better systems will also provide methods for integrating additional training as you work with the system. They provide tools for correcting the errors, and track the errors and corrections, and integrate them into the profile. The level of ease of use and sophistication of this ongoing training is one of the things that separate the quality of the packages. With a motion impaired user, what method and mechanics a given system uses may have a high impact (positive or negative) on how effective the system is long range.
Also in the "training" axis would be the ability to add vocabulary. In a specialized application like microscopy, this would be very important.
I'd also add that technology is changing fast. Look at the revision history of any product you're considering. If it seems static, I would suggest that you do NOT consider this as "stable" (and hence a positive thing) in this application. Programming techniques are changed rapidly, and software that is slow to adapt will be "behind".
I realize that I didn't provide much specific help, but I hope the background helps.
John W. Raffensperger, Jr. IS Manager Helwig Carbon Products, Inc.
-----Original Message----- } From: John J. Bozzola [mailto:bozzola-at-siu.edu] Sent: Tuesday, September 17, 2002 3:26 PM To: Microscopy-at-sparc5.microscopy.com
I apologize is this is not strictly a microscopy question. A microscopist colleague/friend of mine is interested in purchasing a high quality speech recognition software. The individual is handicapped and does not full use of their hands and would be using the software for scientific writing (primarily describing microscopy findings). Although I favor the Macintosh system (since they would also use the computer for image processing and publishing), I am looking for the best software to assist this individual. Any recommendations would be appreciated. Many thanks.
JB
############################################################## John J. Bozzola, Ph.D., Director I.M.A.G.E. (Integrated Microscopy & Graphics Expertise) 750 Communications Drive - MC 4402 Southern Illinois University Carbondale, IL 62901 U.S.A. Phone: 618-453-3730 Fax: 618-453-2665 Email: bozzola-at-siu.edu Web: http://www.siu.edu/~image/ ##############################################################
Tobias is correct that RuO4 will stain such rubbers. Unfortunately, RuO4 is not a selective stain the either the rubber or polystyrene components of HIPS (stains both heavily). OsO4, on the other hand, will stain only the unsaturated polybutadiene of HIPS. I think that you will find OsO4 much more useful.
Regards,
Gary M. Brown ExxonMobil Chemical Company Baytown Polymers Center 5200 Bayway Drive Baytown, Texas 77520-2101 phone: (281) 834-2387 fax: (281) 834-2395 e-mail: Gary.M.Brown-at-ExxonMobil.com
Tobias Baskin {BaskinT-at-missou To: microscopy-at-sparc5.microscopy.com, Debby ri.edu} Sherman {dsherman-at-purdue.edu} cc: Subject: Re: OS staining of rubber 09/19/02 03:16 PM
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Debbie, There is some literature suggesting that ruthenium tetroxide is better than osmium for this kind of thing. There is a paper by Trent, Scheinbeim, and Couchaman 1983 Macromols 16: 589-598 that is very informative. My understanding is that it is usual to vapor stain this kind of sample. Hope this helps, Tobias } } } } Listers, } We, being non-material people, need some help with a material sample. } The sample is a high impact polystyrene (HIPS) that contains butadiene } rubber moieties. We need to be able to identify the location of these } rubber moieties and understand that they will stain upon exposure to osmium. } Does anyone have any experience with this type of sample. Would it be } advisable to stain by floating thin sections (on grids) on liquid osmium or } by using osmium vapors? What type of grids would be most desirable to } minimize corrosion by the osmium? } } Also, we have a diamond knife made by Diatech in Tennessee. I need to } contact them to obtain information about this knife. Does anyone have a } phone number or other contact information? } } Debby } } Debby Sherman, Manager Phone: 765-494-6666 } Life Science Microscopy Facility FAX: 765-494-5896 } Purdue University E-mail: dsherman-at-purdue.edu } S-052 Whistler Building } West Lafayette, IN 47907
Debby, We routinely examine HIPS material in the TEM. Our method is to stain the trimmed and faced sample block in liquid Osmium solution (2% aq) before sectioning. Just place the block in a sealed bottle of solution, only enough to cover is needed, and leave in your hood overnight. Remove in the morning into a small bottle of tap water in the hood for 5 minutes or so, then set the block out in the hood to air dry for a half hour or so. The block should be much darker. Room temperature section as you normally would. Make a careful approach, because the stain will only penetrate for on the order of 10 sections -at- 100nm. 70nm to 90nm sections look very good. HIPS stains very well with this method. Some HIPS samples will warp, making approach more difficult, but usually only to an annoying rather than catastrophic degree. If you have problems, please contact me off-list about recalcitrant samples. Sincerely, Matt
Matthew K. Stephenson Analytical Associate Impact Analytical 1910 West Saint Andrews Road Midland, MI 48640 (989) 832-5555 X506 stephenson-at-impactanalytical.com
I would completely agree with your point about high resolution film etc if we are talking about TEM. In TEM, image forming electrons directly interact with film. So, the quality of the film is a 'limitation factor' there. In TEM even now the film has some advantages over the digital camera. The film greatest advantage - as you mentioned in your message, is ability to enlarge the image without serious pixelation.
In SEM, image forming electrons are detected by some sort of device ("detector"). So, at the output you have actually electrical signal, which represents the properties of your sample. This electrical signal then converted back into the image on the CRT. You also may project CRT image on the film and have a "hard" copy. In such scenario, the image resolution on the film dependent from the quality of the "projection system" and actual size of the SEM probe. Because, signal already present in the "electrical form" (analog or digital) there is no reason to convert it into the image on the film: with modern image grabbers and high-quality printers you may directly convert it into hard copy without intermediate (film) step. In my point of view, this is fundamental difference between SEM and TEM.
Another point, on the film, you could record about 100 shades of gray (dynamic range is 10^2), modern digital devices will record 3-6K levels of grey from the same sample. So, using film in SEM - you lost information, because original signal was (and is) an electronic and then converted into the image. When you directly print your image (digitally) you also loose the dynamic range BUT: you'll still have the original digital image with all that 6K shades of gray. Using film you automatically reduce the dynamic range and, also, keep in mind that film is not linear: it records image in the logarithmic scale... I am sorry... I don't see ANY advantages of using film in SEM, but I DO see some advantages of using film in TEM. Have a good day. Sergey
At 08:45 AM 9/20/02 -0500, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Sergey Ryazantsev, Ph.D. Electron Microscopy Department of Biological Chemistry, School of Medicine University of California, Los Angeles Box 951737 Los Angeles, CA 90095-1737
Hi All, I was contacted by a Post-Doctoral fellow who is seeking a part-time technical position in an EM lab in the NYC area. Her CV is available upon direct request to her. Please respond to her directly, off-line. Lee
ljiljan minwalla, PhD email: minwal01-at-med.nyu.edu -- Leona Cohen-Gould, M.S. Sr. Staff Associate Director, Electron Microscopy Core Facility Manager, Optical Microscopy Core Facility Joan & Sanford I. Weill Medical College of Cornell University voice (212)746-6146 fax (212)746-8175
Most States do not have specific requirements for SF6 handling as it is classed as an inert gas. However it is an asphyxiant and will settle to the floor replacing oxygen. Therefore any labs with a significant amount of SF6 (T tank or more) should be well ventilated with a floor level vent to the outside of the building. In general EM labs tend to be small and not that well ventilated at ground level. In our case we have 3.5" pipe at ground level, near the tank storage and HT generator, tied into a fume hood plenum which has a fan capable of sufficient draught to remove any SF6 spilled.
It does have hazardous decomposition products either generated by electric arcs (SF4, SOF2, SO2F2, OF2 and HF) or heating in the presence of steels which act as a catalyst above 200degC (SF2, SF4, S2F10), however in the quantities used, contained, in microscopy the potential for generation of hazardous byproducts is small.
Regards
Alan
At 01:08 PM 9/19/2002 -0400, Mick Thomas wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Alan W Nicholls, PhD Director of Research Service Facility (Electron Microscopy) Research Resources Center - East (M/C 337) Room 100 Science and Engineering South Building The University of Illinois at Chicago 845 West Taylor St Chicago, IL 60607-7058
We had a large pit under the now-decommissioned HVEM here at Argonne. The pit had a sensor to detect oxygen levels. If the oxygen level dropped below a set point an exhaust fan was started and a warning horn sounded. You shouldn't have to do that. As Greg has pointed out, you'd have to be prone on the floor - face down - before you'd be asphyxiated by the typical setup these days. Nevertheless, you might want to have a small exhaust fan to the building exterior installed at floor level so that you can eliminate as much SF6 as possible in the event of a serious leak. Talk to your institutional safety people.
We also have 1 inch copper pipes installed in the microscope rooms to exhaust/dump SF6 to the building exterior before servicing acceleration chambers or HV tanks. The outlet of the pipes are about 3 to 4 feet above the ground and have a perforated cap to keep out insects. We've also posted warning signs near the outlets.
Russell E. Cook, Ph.D. Electron Microscopy Center Argonne National Laboratory Materials Science Division, Building 212 9700 South Cass Avenue Argonne, IL 60439-4838 (630)252-7194 FAX: (630)252-4289 recook-at-anl.gov } ----------------------------------------------------------------------- } Date: Fri, 20 Sep 2002 08:27:38 -0500 } Subject: RE: SF6 safety } From: Greg Mulhollan {mulhollan-at-extremedevices.com} } } Mick Thomas was inquiring about SF6 safety. Ah, that brings back such } fond memories. Back in my days at SLAC, we were using SF6 as the high } voltage insulating gas for our polarized electron gun. We spent a good } deal of time determining risk levels since the gun operated in a } relatively unventilated underground tunnel separated from the other } sections of the accelerator by large doors. Here are a few of the items } we determined: } 1. SF6 is an asphyxiant and not a poison. In its pure form it is pretty } unreactive. } 2. SF6 is quite heavy and will immediately sink to floor level if there } are in intervening flow barriers. You can consider SF6 as being trapped } somewhere if you think of the analogous amount of water being poured } from or contained in a vessel. In other words, if you have a big vessel } filled with SF6 and open the top, it will retain a good deal of the SF6 } for quite some time and still contain very little oxygen! } 3. Filling our gun injector room with one complete large bottle of SF6 } resulted in only about one inch of an oxygen depleted layer at floor } level. } 4. SF6 after having been in the presence of high voltage arcing, will } break down forming some pretty nasty fluorimers, but generally at low } concentrations. } } In summary: SF6, due to its weight and (usual) inert qualities presents } little risk, except if it is trapped in something or is broken down to } its sub-components. Hope that helps. } } Greg M. } } } Fellow microscopists, } } } } I would be very grateful if someone could offer me advice on how to } } ensure that a microscopy room is set up to safely handle a leak of } SF6. } } } } Thank you very much for your time and help. } } } } Sincerely, } } } } Mick } } } } ------------------------------------------------- } } Mick Thomas } } UHV-STEM Laboratory } } E-1 Clark Hall } } Cornell University } } Ithaca, NY 14853 } } } } Gregory Mulhollan, Ph.D. } Senior Scientist } Extreme Devices Inc. } 3500 ComSouth Drive } Austin, TX 78744 } (512)439-3512 voice } (512)439-3487 fax } mulhollan-at-extremedevices.com }
The standard way to clean molybdenum apertures is in a high vacuum coating unit, heating the apertures to orange-red and holding them at that temperature until the deposit(s) evaporate.
Heating in a sputter coater or in a flame does not work with molybdenum. Heating to white heat is not a good idea as this often distorts the aperture or, if you try to re use the cleaned apertures and clean them again grain growth also tends to spoil the aperture shape.
If you are unable to clean the apertures by the first method described you are better off discarding them; dirty apertures are not a good idea!
Steve Chapman Senior Consultant Protrain For consultancy and professional training in EM world wide Tel 44+ 1280 814774 Direct Line 816512 Fax 814007 www.emcourses.com
I have had someone come to me asking about microscopic methods of reading data on hard disk platters. Does anyone have experience along these lines, or suggestions of who may have done this sort of thing? The question seems to deal mainly with the persistence of the magnetic domains, and what sort of 'memory' the disk maintains during multiple writing operations.
Any suggestions would me greatly appreciated.
Ben Simkin (simkin-at-egr.msu.edu) Michigan State University
I have uncovered a box ~4x5x2 in that looks like an exposure device for a Nikon photomicroscope. It has selections for manual/auto, speed, ASA, time, and over/under adjustments. It has a cord that fastens to the camera with 8 pins around the periphery and 2 in the center. If anyone can use it, I will mail it. Otherwise it goes into the dump.
Sara E. Miller, Ph. D. P. O. Box 3712 Duke University Medical Center Durham, NC 27710 Ph: 919 684-3452 FAX: 919 684-3265
How many JEOL 2010Fs are there out there? If you have one I would appreciate it if you would drop me a line directly and not to the list. Thanks.
-- John Mansfield PhD MInstP North Campus Electron Microbeam Analysis Laboratory 417 SRB, University of Michigan 2455 Hayward, Ann Arbor MI 48109-2143 Phone: (734) 936-3352 FAX (734) 763-2282 Cell. Phone: (734) 834-3913 (Leaving a phone message at 936-3352 is preferable to 834-3913) Email: jfmjfm-at-engin.umich.edu URL: http://emalwww.engin.umich.edu/people/jfmjfm/jfmjfm.html Location: Lat. 42! 16' 48" Long. 83! 43' 48"
If the apertures are from a Philips TEM, they are most likely made of Platinum. You don't heat these in vacuum as you do the Mo apertures. These can be cleaned by heating them in a Pt basket over a bunsen burner in air. The oxygen in air won't oxidize the Pt, but will remove the hydrocarbon contamination quite effectively.
If you look in your CM12 owners book, Philips should have a section on maintenance where they describe the procedure.
Cheers, Henk Colijn
At 08:30 AM 9/20/2002 +0200, =?ISO-8859-2?Q?Old=F8ich_Benada?= wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Hendrik O. Colijn colijn.1-at-osu.edu Campus Electron Optics Facility Ohio State University (614) 292-0674 http://www.ceof.ohio-state.edu Fools are pleased when they discover error. The wise are pleased when they discover truth.
Ann and others, I am glad that you have found the MSA Facility Management series useful. Unfortunately it may be held less often in the future. Due to the large number of annually repeating sessions that limit addition of new sessions, it looks like it will be relegated to every other year starting immediately although there is no guarantee that it will be continued in the future. At least there will be no support yearly so speakers will have to be gleaned from those already going to the meetings. This is usually the case for most anyway but has not been the case for all. We will try to limp along if we can find appropriate facilitators already going to the meeting and a room to hold the session. Hopefully we will still get funding for the audio-visual required. In any case let's be optimistic and plan on a session at M&M2003. With that, I have a few ideas as a topic but, since this is meant to be relative to all you lab managers out there, what would you like to have presented/discussed at the next session? Please let me know with suggestions for facilitators as well.
Debby
On 9/20/02 11:32 AM, "Lehman, Ann" {Ann.Lehman-at-trincoll.edu} wrote:
} Hi Debbie, } } Many moons ago (in the 80's) I regularly used Kodak Ektapan sheet film in } 4x5 carriers inserted into the Polaroid holder, and got good results. Tech } Pan sounds promising though. } } I can appreciate your desire to get good negatives, as I am struggling with } an intro SEM course in which my students are only exposed to digital imaging } (no pun intended). I feel I am short-changing them. } } Let us know what you learn!! } } And thanks again for organizing the MSA facility management series. } } cheers, } Ann } } ################### } Ann Hein Lehman } Assistant Director, EM Facility } Trinity College - LSC314 } 300 Summit Street } Hartford CT 06106 } v. 860-297-4289 } f. 860-297-2538 } e. ann.lehman-at-trincoll.edu } w. http://www.trincoll.edu/~alehman/ } Facility beta: http://www.trincoll.edu/~alehman/EM_Facility.htm }
Dear Debby, The limitation of resolution from an SEM image is not the fine grain of the film, but the line resolution of the SEM and photo CRT and the ability of the photo CRT and camera to resolve those lines. While you can enlarge a TEM image ten times because the image is a real image and the film can still resolve features at that enlargement, the SEM image will start to show you the lines in the SEM CRT above about five times enlargement. If you do not see the lines, then your SEM CRT is not focussing even that well and your image will be degraded further. Fine film won't help that. The highest resolution SEM photo CRT I have seen is 2500 lines and so that is the most lines that the SEM will put out. There is no reason that a 2500 line image from the film camera is going to be any better or sharper or higher resolution than a 2500 line digital image. The only choice is the output media and, with glossy photo paper, an high-resolution inkjet printer will give you a two minute 8 X 10 print. There is nothing magic about film or inferior about digital imaging. At 08:45 AM 09/20/2002 -0500, you wrote:
} Listers, } I arrived at work today to find a number of responses to my earlier post } asking about film for SEM. I have listed them below without reference to } sender. } I also had a number of responses asking why I wanted to use film for } SEM. This is a good question since for 99% of our SEM work we do capture } digital images and they are adequate for most purposes. However, I guess I } am still from the old school. I still find film better than digital if you } want to enlarge images. } In this particular case, we are hoping to purchase a high resolution } FESEM. A goodly percentage (not all) of the samples will be very } small...things like viruses, liposomes, and various nanoparticles with sizes } ranging from 10nm up. Although the newest models of FESEM can resolve these } structures, even though we will also have to deal with cryo conditions as } most samples will be hydrated, there is still the problem of "empty } magnification" when taking the original image. This limit to the useful } magnification when we originally capture the image is the potential problem. } In many cases we envision that we may need to substantially enlarge } single particles to illustrate finer features to our audience. In this } case, using very fine grained film will give us more opportunity to increase } size without concern for pixelization or without having a computer decide } how to insert smaller pixels (as would happen if we just punch in a higher } resolution figure and let the computer interpret). In fact, it surprises me } that for a relatively small sum when considering the cost of the entire } instrument package, many people do not choose to have the option of using } film when purchasing a new high resolution instrument. You may never use it } but you may well wish to have the option sometime down the road. } } Again, thanks to all who responded. I may get a few more responses as } the day goes on but wanted to get this off before it gets buried in my in } box. As to final choice of film....I plan to try a number of the suggested } ones and see what fits our needs. } } Debby } ..snip
Regards, Mary
Mary Mager Electron Microscopist Metals and Materials Engineering University of British Columbia 6350 Stores Road Vancouver, B.C. V6T 1Z4 CANADA tel: 604-822-5648 e-mail: mager-at-interchg.ubc.ca
Several years ago (4-5) we looked at this issue in regards to handling rodent filth & concerns about hantavirus, etc. From the literature search we found the following (which may have changed) when looking at latex vs. nitrile gloves:
1. No known allergic reactions to nitrile. 2. Nitrile gloves had smaller pores than latex gloves. 3. Nitrile gloves had a lower failure rate during testing than latex gloves.
We switched to nitrile gloves for "filth" work.
These are my own comments & not of my employer. David A. Foran, chemist Food and Drug Administration Kansas City Elemental Analysis Lab DFORAN-at-ORA.FDA.GOV 913-752-2170 913-752-2727 (voice mail) 913-752-2151 (fax)
-----Original Message----- } From: "Frida.Maiers-at-co.hennepin.mn.us"-at-sparc5.microscopy.com [mailto:"Frida.Maiers-at-co.hennepin.mn.us"-at-sparc5.microscopy.com] Sent: Wednesday, September 18, 2002 1:30 PM To: microscopy-at-sparc5.microscopy.com
The shutter control has found a home.
Sara E. Miller, Ph. D. P. O. Box 3712 Duke University Medical Center Durham, NC 27710 Ph: 919 684-3452 FAX: 919 684-3265
It gets worse than that : c.a. 1985 when working on a SEM in a colleagues lab I noticed that the horizontal scan lines that were normally distinguishable at certain faster scan settings on my instrument were not visible on his (same mfg., same scan module, same recording CRT, different chamber and spectrometer setup). When I inquired, he told me that the mfg.'s service rep had been there only the day before and completely optimized everything, including readjusting the brightness and contrast settings on the recording CRT.
After a little investigation I found that the tech had decreased the brightness settings and compensated by opening the photo transfer lens iris from f-8 to f-5.6. I had already learned from experience that an iris opening this wide led to a a defocused image of the CRT spot on the film which could not be corrected by any adjustment of the mechanical focus.
When asked why he had intentionally defocused the image, the tech responded that the faintly visible scan lines on fast frame rates annoyed some customers so he made them happy by effectively blurring the image so that the raster lines ran together!!! (Names withheld to protect the guilty)
Part of the point of this story is that the vertical resolution on a SEM may be limited by the number of lines in the raster pattern rather than the film or the camera system. On a high resolution CRT with type 55 P/N film the individual lines were often discernable. However, the horizontal resolution is limited only by the instrument response factors, imaging conditions and the film. To ensure that optimal resolution is maintained, one may have to live with some raster artifacts in the vertical direction if, for example, a fast scan rate is required due to an unstable sample.
John Twilley Conservation Scientist
Mary Mager wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } Dear Debby, } The limitation of resolution from an SEM image is not the fine grain of the } film, but the line resolution of the SEM and photo CRT and the ability of } the photo CRT and camera to resolve those lines. While you can enlarge a } TEM image ten times because the image is a real image and the film can still } resolve features at that enlargement, the SEM image will start to show you } the lines in the SEM CRT above about five times enlargement. If you do not } see the lines, then your SEM CRT is not focussing even that well and your } image will be degraded further. Fine film won't help that. The highest } resolution SEM photo CRT I have seen is 2500 lines and so that is the most } lines that the SEM will put out. There is no reason that a 2500 line image } from the film camera is going to be any better or sharper or higher } resolution than a 2500 line digital image. The only choice is the output } media and, with glossy photo paper, an high-resolution inkjet printer will } give you a two minute 8 X 10 print. There is nothing magic about film or } inferior about digital imaging.
The ability of film to record SEM or TEM data has to be compared to the scan rate density of SEM (2K) and TEM (integrated) versus that of the actual film's capabilities.
A finer grain film in a SEM environment at 2K lpi is not going to be all that impressive compared to a direct digital capture at 4Kx4K. the other factor in favor of digital capture is realtime evaluation of the histogram of the total image. One can optimize contrast and brightness to collect a perfect image. Using film, this is hit or miss at best.
gary g.
At 03:07 PM 9/20/2002, you wrote:
} Ann and others, } I am glad that you have found the MSA Facility Management series useful. } Unfortunately it may be held less often in the future. Due to the large } number of annually repeating sessions that limit addition of new sessions, } it looks like it will be relegated to every other year starting immediately } although there is no guarantee that it will be continued in the future. At } least there will be no support yearly so speakers will have to be gleaned } from those already going to the meetings. This is usually the case for most } anyway but has not been the case for all. } We will try to limp along if we can find appropriate facilitators } already going to the meeting and a room to hold the session. Hopefully we } will still get funding for the audio-visual required. } In any case let's be optimistic and plan on a session at M&M2003. With } that, I have a few ideas as a topic but, since this is meant to be relative } to all you lab managers out there, what would you like to have } presented/discussed at the next session? Please let me know with } suggestions for facilitators as well. } } Debby } } } } On 9/20/02 11:32 AM, "Lehman, Ann" {Ann.Lehman-at-trincoll.edu} wrote: } } } Hi Debbie, } } } } Many moons ago (in the 80's) I regularly used Kodak Ektapan sheet film in } } 4x5 carriers inserted into the Polaroid holder, and got good results. Tech } } Pan sounds promising though. } } } } I can appreciate your desire to get good negatives, as I am struggling with } } an intro SEM course in which my students are only exposed to digital } imaging } } (no pun intended). I feel I am short-changing them. } } } } Let us know what you learn!! } } } } And thanks again for organizing the MSA facility management series. } } } } cheers, } } Ann } } } } ################### } } Ann Hein Lehman } } Assistant Director, EM Facility } } Trinity College - LSC314 } } 300 Summit Street } } Hartford CT 06106 } } v. 860-297-4289 } } f. 860-297-2538 } } e. ann.lehman-at-trincoll.edu } } w. http://www.trincoll.edu/~alehman/ } } Facility beta: http://www.trincoll.edu/~alehman/EM_Facility.htm } }
This also brings back some not so fond memories of SF6 for a HVEM microscope where is was used in the high voltage tanks. When we had to open the tanks for service, the gas had to be pumped into underground storage tanks. When we were finished with the repairs, the SF6 was pumped back into the accelerator and generator through molecular sieve to remove moisture. This meant that I had to then vacuum the filters to remove the powdered molecular sieve material formed as the gas blasted through them. From the noise it may be been at supersonic speeds, at least to begin with. I think that the powdered molecular sieve dust can be dangerous to breathe into your lungs and it gets everywhere and when vacuuming I had to ground myself, the vacuum and the filter holder.
Damian Neuberger.
} Mick Thomas was inquiring about SF6 safety. Ah, that brings back such } fond memories. Back in my days at SLAC, we were using SF6 as the high } voltage insulating gas for our polarized electron gun. We spent a good } deal of time determining risk levels since the gun operated in a } relatively unventilated underground tunnel separated from the other } sections of the accelerator by large doors. Here are a few of the items } we determined: } 1. SF6 is an asphyxiant and not a poison. In its pure form it is pretty } unreactive. } 2. SF6 is quite heavy and will immediately sink to floor level if there } are in intervening flow barriers. You can consider SF6 as being trapped } somewhere if you think of the analogous amount of water being poured } from or contained in a vessel. In other words, if you have a big vessel } filled with SF6 and open the top, it will retain a good deal of the SF6 } for quite some time and still contain very little oxygen! } 3. Filling our gun injector room with one complete large bottle of SF6 } resulted in only about one inch of an oxygen depleted layer at floor } level. } 4. SF6 after having been in the presence of high voltage arcing, will } break down forming some pretty nasty fluorimers, but generally at low } concentrations. } } In summary: SF6, due to its weight and (usual) inert qualities presents } little risk, except if it is trapped in something or is broken down to } its sub-components. Hope that helps.
Twenty years ago I helped design an SEM for IBM's storage products division in Rochester, MN (I don't think they exist anymore, at least not there). This was back in the days of the 12" platters and this instrument was designed to enable imaging of any portion of the disk at high tilt angles (biggest sample chamber ever made, as far as I know).
Having said that, I have to question the source of the question. Recovering data from hard drives that has been written over is really only done for one legitimate reason - law enforcement, and one perhaps self-legitimizing reason - intelligence gathering. Data recovery services would not normally attempt anything so esoteric, and customers don't come to them for recovering such data. They generally handle bad drive controller electronics and head crashes that have destroyed sector data - wanting to recover recent data. There is no data that an individual would have that would be worth the effort, even if they lost business informat ion. Far easier and less expensive to reconstruct it by other means.
With that head's up, I'll just say that the positioning of the heads is not perfect. They do not write over the exact same area every time. The persistence of the domains is very long under normal operating conditions. Finding the anomalies and producing a coherent representation of the underlying data is the problem - it's not easy and the ability to reproduce sizable chunks of data depends on many variables.
Allen R. Sampson Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174
On Friday, September 20, 2002 1:47 PM, "simkin-at-egr.msu.edu"-at-sparc5.microscopy.com [SMTP:"simkin-at-egr.msu.edu"-at-sparc5.microscopy.com] wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Hi all, } } I have had someone come to me asking about microscopic methods of reading } data on hard disk platters. Does anyone have experience along these lines, } or suggestions of who may have done this sort of thing? The question seems to } deal mainly with the persistence of the magnetic domains, and what sort of } 'memory' the disk maintains during multiple writing operations. } } Any suggestions would me greatly appreciated. } } Ben Simkin (simkin-at-egr.msu.edu) } Michigan State University } } } }
I'm not going to argue the merits of digital vs. analog at this point. Gary's point about the histogram has caught my interest.
Many SEM's offer the ability to view an analog 'waveform' (each manufacturer seems to call it by a different name). This is essentially an oscillographic display of the signal intensity. It is a dynamic display of each scan line's signal as opposed to the static histogram of most image capture systems which offer a representation of the sum of all scan lines. The difference is that an accomplished operator may adjust the brightness and contrast to a particular feature of interest, rather than the total frame. You could put a digital system in line mode and manually run the line position up and down to characterize the feature of interest, but with the waveform display you can see this with every frame, as well as the overall signal frame response.
Just a thought.
Allen R. Sampson Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174
On Friday, September 20, 2002 7:48 PM, Gary Gaugler [SMTP:gary-at-gaugler.com] wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } The ability of film to record SEM or TEM data has to be compared } to the scan rate density of SEM (2K) and TEM (integrated) versus } that of the actual film's capabilities. } } A finer grain film in a SEM environment at 2K lpi is not going to } be all that impressive compared to a direct digital capture at } 4Kx4K. the other factor in favor of digital capture is realtime } evaluation of the histogram of the total image. One can optimize } contrast and brightness to collect a perfect image. Using film, this } is hit or miss at best. } } gary g. } } } At 03:07 PM 9/20/2002, you wrote: } } } Ann and others, } } I am glad that you have found the MSA Facility Management series useful. } } Unfortunately it may be held less often in the future. Due to the large } } number of annually repeating sessions that limit addition of new sessions, } } it looks like it will be relegated to every other year starting immediately } } although there is no guarantee that it will be continued in the future. At } } least there will be no support yearly so speakers will have to be gleaned } } from those already going to the meetings. This is usually the case for most } } anyway but has not been the case for all. } } We will try to limp along if we can find appropriate facilitators } } already going to the meeting and a room to hold the session. Hopefully we } } will still get funding for the audio-visual required. } } In any case let's be optimistic and plan on a session at M&M2003. With } } that, I have a few ideas as a topic but, since this is meant to be relative } } to all you lab managers out there, what would you like to have } } presented/discussed at the next session? Please let me know with } } suggestions for facilitators as well. } } } } Debby } } } } } } } } On 9/20/02 11:32 AM, "Lehman, Ann" {Ann.Lehman-at-trincoll.edu} wrote: } } } } } Hi Debbie, } } } } } } Many moons ago (in the 80's) I regularly used Kodak Ektapan sheet film in } } } 4x5 carriers inserted into the Polaroid holder, and got good results. Tech } } } Pan sounds promising though. } } } } } } I can appreciate your desire to get good negatives, as I am struggling with } } } an intro SEM course in which my students are only exposed to digital } } imaging } } } (no pun intended). I feel I am short-changing them. } } } } } } Let us know what you learn!! } } } } } } And thanks again for organizing the MSA facility management series. } } } } } } cheers, } } } Ann } } } } } } ################### } } } Ann Hein Lehman } } } Assistant Director, EM Facility } } } Trinity College - LSC314 } } } 300 Summit Street } } } Hartford CT 06106 } } } v. 860-297-4289 } } } f. 860-297-2538 } } } e. ann.lehman-at-trincoll.edu } } } w. http://www.trincoll.edu/~alehman/ } } } Facility beta: http://www.trincoll.edu/~alehman/EM_Facility.htm } } } } } } }
The person whom I received the question from is an old childhood friend with a strong curiosity. He is one of the computer geeks for a local programming concern. The thing that piqued his interest was an assertion that it required a minimum of 7 writing cycles to obscure old drive data, so he wants to test it. I confess myself surprised by this, so now I'm interested as well. I would not have expected much of anything to have survived more than 3 writes. I find myself wondering if (beyond track wander) there is less than perfect flipping of domains in the entire area of a bit. (Of course I could be way out on a limb here because this is isn't my area of expertise by a long shot.)
Ben Simkin (simkin-at-egr.msu.edu) Michigan State University
} Twenty years ago I helped design an SEM for IBM's storage products division } in Rochester, MN (I don't think they exist anymore, at least not there). } This was back in the days of the 12" platters and this instrument was } designed to enable imaging of any portion of the disk at high tilt angles } (biggest sample chamber ever made, as far as I know). } } Having said that, I have to question the source of the question. } Recovering data from hard drives that has been written over is really only } done for one legitimate reason - law enforcement, and one perhaps } self-legitimizing reason - intelligence gathering. Data recovery services } would not normally attempt anything so esoteric, and customers don't come } to them for recovering such data. They generally handle bad drive } controller electronics and head crashes that have destroyed sector data - } wanting to recover recent data. There is no data that an individual would } have that would be worth the effort, even if they lost business informat } ion. Far easier and less expensive to reconstruct it by other means. } } With that head's up, I'll just say that the positioning of the heads is not } perfect. They do not write over the exact same area every time. The } persistence of the domains is very long under normal operating conditions. } Finding the anomalies and producing a coherent representation of the } underlying data is the problem - it's not easy and the ability to reproduce } sizable chunks of data depends on many variables. } } } Allen R. Sampson } Advanced Research Systems } 317 North 4th. Street } St. Charles, Illinois 60174 } } phone (630) 513-7093 fax (630) 513-7092 http://www.sem.com } } } } Hi all, } } } } I have had someone come to me asking about microscopic methods of } reading } } data on hard disk platters. Does anyone have experience along these } lines, } } or suggestions of who may have done this sort of thing? The question } seems to } } deal mainly with the persistence of the magnetic domains, and what sort } of } } 'memory' the disk maintains during multiple writing operations. } } } } Any suggestions would me greatly appreciated. } } } } Ben Simkin (simkin-at-egr.msu.edu) } } Michigan State University
We work on disk platter and head everyday. It is impossible to "see" magnetic domain on optical microscope, neither SEMs. On a disk with data density of 10-20GB/side of platter, the width of track is ~0.4 um and simular scale on the length, the thickness of magnetic layer is 10-30 nm. It is too small for optical microscope and too thin for SEM to get enough mass (for holding magnetic energy) for SEI signal.
AFM with magnetic tip is one good tool to see the magnetic field image (field distribution map). Another instrument, call Optical Surface Analyzer (OSA) is another good choice to see the magnetic domain. The resolution can not reach single domain, just see the data stream as noise waveform.
When you open a hard drive without clean toom envionment, the surface of disk would be contaminated by floating particles (dust). You will no longer be able to see the original surface.
Zhiyu Wang Maxtor Corp. zhiyu_wang-at-maxtor.com
----- Original Message ----- } From: {"simkin-at-egr.msu.edu"-at-sparc5.microscopy.com} To: {Microscopy-at-sparc5.microscopy.com} Sent: Friday, September 20, 2002 8:47 PM
Suppose, just suppose, that a magnetic head does not do a complete job of magnetizing a particular group of grains in the thin film of a hard drive disk - it does, however, change it enough to be recognizable when that portion is read. If the film had at first been completely demagnetized, the first write would leave it at some percentage of complete polarization. A second write at that site would then leave one of two states - augmentation of the original write if the polarity was the same or a reversal of polarity. In the first case, the group has a slightly higher magnetization in the same direction, in the latter a slightly lessor magnetization in the opposite direction. Double those two states since there are two polarities to the magnetic charge, and you have four separate possible states.
When a third write operation is made, eight different states could be imagined. In the case where the write is of the same polarity as the first and second, the magnetization is again enhanced. When the current write opposes the previous two, the group is left at a lower state of opposite polarity. If the current write opposes the previous write which opposed the first write, the magnetization is lessened and opposite in polarity. And finally, if the current write is of the same polarity as the previous write and opposite of the first write, the previous state is enhanced. Once again, double those states as we are dealing with two polarization states.
While it may seem from the above that there is a continuing reduction in the magnetic charge, statistically there is a 50% chance that any particular write will increase the magnetic charge, so in the long run there is a predictable magnetic charge, in either polarity, on this group of magnetic grains, and thus a reliable level at which one can determine the difference between states of the last write.
The question really becomes one of the resolution available to read these individual charges and the amount of computational power available to deconvolute the possible states. Three writes is generally enough to satisfy the normal paranoid personality. For those concerned with the black helicopters outside their windows and nightmares of NSA, seven writes may suffice. But the technology of US government agencies should never be underestimated.
Why this situation might occur is a question of economics and physics. We want the most data storage available per linear unit of hard drive space. There is an overlap between what works reliably and what leaves detectable traits.
Allen R. Sampson Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174
On Saturday, September 21, 2002 7:05 PM, "simkin-at-egr.msu.edu"-at-sparc5.microscopy.com [SMTP:"simkin-at-egr.msu.edu"-at-sparc5.microscopy.com] wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Just some further information to settle fears- } } The person whom I received the question from is an old childhood friend with } a strong curiosity. He is one of the computer geeks for a local programming } concern. } The thing that piqued his interest was an assertion that it required a } minimum of 7 writing cycles to obscure old drive data, so he wants to test it. } I confess myself surprised by this, so now I'm interested as well. I would } not have expected much of anything to have survived more than 3 writes. } I find myself wondering if (beyond track wander) there is less than perfect } flipping of domains in the entire area of a bit. (Of course I could be way out } on a limb here because this is isn't my area of expertise by a long shot.) } } Ben Simkin (simkin-at-egr.msu.edu) } Michigan State University } } } } } Twenty years ago I helped design an SEM for IBM's storage products division } } in Rochester, MN (I don't think they exist anymore, at least not there). } } This was back in the days of the 12" platters and this instrument was } } designed to enable imaging of any portion of the disk at high tilt angles } } (biggest sample chamber ever made, as far as I know). } } } } Having said that, I have to question the source of the question. } } Recovering data from hard drives that has been written over is really only } } done for one legitimate reason - law enforcement, and one perhaps } } self-legitimizing reason - intelligence gathering. Data recovery services } } would not normally attempt anything so esoteric, and customers don't come } } to them for recovering such data. They generally handle bad drive } } controller electronics and head crashes that have destroyed sector data - } } wanting to recover recent data. There is no data that an individual would } } have that would be worth the effort, even if they lost business informat } } ion. Far easier and less expensive to reconstruct it by other means. } } } } With that head's up, I'll just say that the positioning of the heads is not } } perfect. They do not write over the exact same area every time. The } } persistence of the domains is very long under normal operating conditions. } } Finding the anomalies and producing a coherent representation of the } } underlying data is the problem - it's not easy and the ability to reproduce } } sizable chunks of data depends on many variables. } } } } } } Allen R. Sampson } } Advanced Research Systems } } 317 North 4th. Street } } St. Charles, Illinois 60174 } } } } phone (630) 513-7093 fax (630) 513-7092 http://www.sem.com } } } } } } } Hi all, } } } } } } I have had someone come to me asking about microscopic methods of } } reading } } } data on hard disk platters. Does anyone have experience along these } } lines, } } } or suggestions of who may have done this sort of thing? The question } } seems to } } } deal mainly with the persistence of the magnetic domains, and what sort } } of } } } 'memory' the disk maintains during multiple writing operations. } } } } } } Any suggestions would me greatly appreciated. } } } } } } Ben Simkin (simkin-at-egr.msu.edu) } } } Michigan State University } } } }
Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (michelle-snyder-at-augustana.edu) from http://www.msa.microscopy.com/Ask-A-Microscopist.html on Sunday, September 22, 2002 at 10:04:10 ---------------------------------------------------------------------------
Organization: St Francis Medical Center School of Clinical Laboratory Science
Education: Graduate College
Location: Peoria, Il, USA
Question: Do you have any idea who could service a Sorvall MT-2 ultra microtome? I am experiencing macroscopic chatter, I am assuming something is wrong with a bearing or the counterweight. I have contacted serveral companies and each gives me another name with no luck...Leica, Kendro, Ventana, Broeckler, etc. Any help would be much appreciated, I just want to get back to sectioning. Thanks so much!
Magnetic domains can also be imaged in a TEM using the technique of Lorentz microscopy. In Lorentz microscopy you work at a very low or zero objective lens excitation so as not to affect the domains. You will have to adjust focus with the z-height if possible. You will also have a scale problem.
You might be able to seen the domains in SEM if you decorate the domains with very fine ferromagnetic particles, a la the Bitter effect. There are also SEMs that have spin polarizing filters that you could use to image the domains.
I believe the US intelligence agencies recommend overwriting and defragmenting your disk seven times. They probably can extract remanent domains that remain after incomplete eraser.
Don Werder
Allen Sampson wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
At 10:05 PM 9/21/2002 -0400, simkin-at-egr.msu.edu"-at-sparc5.microscopy.com wrote: } The person whom I received the question from is an old childhood friend with } a strong curiosity. He is one of the computer geeks for a local programming } concern. } The thing that piqued his interest was an assertion that it required a } minimum of 7 writing cycles to obscure old drive data, so he wants to test it. } I confess myself surprised by this, so now I'm interested as well. I would } not have expected much of anything to have survived more than 3 writes. } I find myself wondering if (beyond track wander) there is less than perfect } flipping of domains in the entire area of a bit.
If your friend did a little digging into the published descriptions of the field of computer forensics, he would find a number of explanations of the techniques and equipment used to recover this phantom data. They don't use SEMs. The re-written data can be recovered in some cases because the magnetized regions are generally larger than the read heads, and ghosts of the past data can be discerned if you examine the trackways with something other than the ordinary read-head.
If you pursue this discussion any further, I suspect you will have violated the new Patriot Act and numerous other laws forbidding discussion of the possibility of maybe uncovering classified data. -Michael
Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (spyker-at-bright.net) from http://www.msa.microscopy.com/Ask-A-Microscopist.html on Sunday, September 22, 2002 at 15:45:54 ---------------------------------------------------------------------------
Email: spyker-at-bright.net Name: lauren
Organization: Perry Jr. High
Education: 6-8th Grade Middle School
Location: Lima, Ohio USA
Question: What is the best way to prepare an insect wing for a slide mount...
on 9/18/02 7:18 PM, Tobias Baskin at BaskinT-at-missouri.edu wrote: } } } Microscopists, } I have a run of Journal of Cell Biology from 1987 through } 2001 that I would like to give away. Our library doesn't want them. } Anyone out there interested? Or know of a connection to libraries } somewhere that might be interested? } Dear Tobias, The American Physical Society has a journal donation program, and the International Center for Theoretical Physics in Trieste will often reimburse the donor for shipping journals to underdeveloped nations. While this may not be appropriate for JCB, there may be similar programs sponsored by biologically-oriented professional societies. Yours, Bill Tivol
on 9/19/02 1:08 PM, Mick Thomas at mgt3-at-ccmr.cornell.edu wrote: } } I would be very grateful if someone could offer me advice on how to ensure } that a microscopy room is set up to safely handle a leak of SF6. } } Thank you very much for your time and help. } } Sincerely, } Dear Mick, SF6 is not, itself, toxic; however, it can displace air, and, since it will settle on the floor, if someone loses consciousness from lack of oxygen, that can be fatal. Furthermore, I was recently told that SF6 can produce F when it decomposes due to, say, a fire. The specifications for SF6 safety are to have an exhaust, preferably located near the floor, which pumps room air directly to the outside--i.e., not into the air conditioning air return, etc. I do not know the air flow requirements, but someone else on the list may have that info. Yours, Bill Tivol
I would like to thank to all who kindly response to my question about cleaning the C2 apertures of CM12. The list of responses can be seen on: http://www.biomed.cas.cz/~benada/c2_aperture_cleaning.htm
Many thanks again. Oldrich
+-----------------------------------+ Oldrich Benada Acad. Sci. CR Institute of Microbiology Laboratory of electron microscopy Videnska 1083 CZ - 142 20 Prague 4 - Krc Czech Republic +------------------------------------+ Phone: +420-2-41062399 Fax: +420-2-41062347 WEB: http://www.biomed.cas.cz/mbu/lem113/lem.htm
After years of using a waveform monitor (what it's called on JEOL scopes) with film, I really missed it on the 5600, even for digital images. Setting brightness and contrast consistently, particularly for critical areas of the image, is much easier with this tool. I missed it so much, I decided to write my own software waveform monitor. See:
http://www.mta.ca/~jehrman/software.htm
Notice: I have a (small) commercial interest here, in that I sell the WFM (and a companion program -LSP- as a filament saturation aid), to augment my rather meager salary here in the Great White North. Using both routinely have given me more consistent and pleasing images, and longer filament life.
Both will work on any Windows based digital instrument, or any imaging software (such as Photoshop) where there is an interest in seeing gray-scale values in a waveform format. Contact me offline if you're interested.
Regards,
Jim Ehrman
Allen Sampson wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } I'm not going to argue the merits of digital vs. analog at this point. } Gary's point about the histogram has caught my interest. } } Many SEM's offer the ability to view an analog 'waveform' (each } manufacturer seems to call it by a different name). This is essentially an } oscillographic display of the signal intensity. It is a dynamic display of } each scan line's signal as opposed to the static histogram of most image } capture systems which offer a representation of the sum of all scan lines. } The difference is that an accomplished operator may adjust the brightness } and contrast to a particular feature of interest, rather than the total } frame. You could put a digital system in line mode and manually run the } line position up and down to characterize the feature of interest, but with } the waveform display you can see this with every frame, as well as the } overall signal frame response. } } Just a thought. } } Allen R. Sampson } Advanced Research Systems } 317 North 4th. Street } St. Charles, Illinois 60174 } } phone (630) 513-7093 fax (630) 513-7092 http://www.sem.com } } On Friday, September 20, 2002 7:48 PM, Gary Gaugler [SMTP:gary-at-gaugler.com] } wrote: } } ------------------------------------------------------------------------ } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } } -----------------------------------------------------------------------. } } } } } } The ability of film to record SEM or TEM data has to be compared } } to the scan rate density of SEM (2K) and TEM (integrated) versus } } that of the actual film's capabilities. } } } } A finer grain film in a SEM environment at 2K lpi is not going to } } be all that impressive compared to a direct digital capture at } } 4Kx4K. the other factor in favor of digital capture is realtime } } evaluation of the histogram of the total image. One can optimize } } contrast and brightness to collect a perfect image. Using film, this } } is hit or miss at best. } } } } gary g. } } } } } } At 03:07 PM 9/20/2002, you wrote: } } } } } Ann and others, } } } I am glad that you have found the MSA Facility Management series } useful. } } } Unfortunately it may be held less often in the future. Due to the large } } } number of annually repeating sessions that limit addition of new } sessions, } } } it looks like it will be relegated to every other year starting } immediately } } } although there is no guarantee that it will be continued in the future. } At } } } least there will be no support yearly so speakers will have to be } gleaned } } } from those already going to the meetings. This is usually the case for } most } } } anyway but has not been the case for all. } } } We will try to limp along if we can find appropriate facilitators } } } already going to the meeting and a room to hold the session. Hopefully } we } } } will still get funding for the audio-visual required. } } } In any case let's be optimistic and plan on a session at M&M2003. } With } } } that, I have a few ideas as a topic but, since this is meant to be } relative } } } to all you lab managers out there, what would you like to have } } } presented/discussed at the next session? Please let me know with } } } suggestions for facilitators as well. } } } } } } Debby } } } } } } } } } } } } On 9/20/02 11:32 AM, "Lehman, Ann" {Ann.Lehman-at-trincoll.edu} wrote: } } } } } } } Hi Debbie, } } } } } } } } Many moons ago (in the 80's) I regularly used Kodak Ektapan sheet } film in } } } } 4x5 carriers inserted into the Polaroid holder, and got good results. } Tech } } } } Pan sounds promising though. } } } } } } } } I can appreciate your desire to get good negatives, as I am } struggling with } } } } an intro SEM course in which my students are only exposed to digital } } } imaging } } } } (no pun intended). I feel I am short-changing them. } } } } } } } } Let us know what you learn!! } } } } } } } } And thanks again for organizing the MSA facility management series. } } } } } } } } cheers, } } } } Ann } } } } } } } } ################### } } } } Ann Hein Lehman } } } } Assistant Director, EM Facility } } } } Trinity College - LSC314 } } } } 300 Summit Street } } } } Hartford CT 06106 } } } } v. 860-297-4289 } } } } f. 860-297-2538 } } } } e. ann.lehman-at-trincoll.edu } } } } w. http://www.trincoll.edu/~alehman/ } } } } Facility beta: http://www.trincoll.edu/~alehman/EM_Facility.htm } } } } } } } } } } } }
--
James M. Ehrman Digital Microscopy Facility Mount Allison University Sackville, NB E4L 1G7 CANADA
CALL FOR NOMINATIONS FOOD STRUCTURE AND FUNCTIONALITY DIVISION ( at AOCS) AWARD
This award honors outstanding lifetime performance and meritorious contributions to an area of interest to the Food Structure & Functionality Division of the American Oil Chemists' Society. The award will be presented during the 94th AOCS annual Meeting & Exp to be held in Kansas City, Missouri, May 4-7, 2003 and consists of $1,500USD to help defray costs incurred by the awardee in participating in the AOCS Annual Meeting & Expo, and also a crystal plaque.
Nominations should consist of a letter of nomination, supporting letters from at least three other scientists, and biographical information concerning the nominee. The biographical information must include a summary of the nominee's research accomplishments, a list of publication, degree(s) held (with the names of granting institutions) and positions(s) held during the nominee's professional career.
For further information on nomination procedures contact the Food Structure & Functionality Division Award Canvassing Committee Chairperson, Dr, Judy Arnold, USDA-ARS_RRC, 950 College Station Rd., P.O. Box 5677, Athens, GA 30604-5677, USA, Tel: 706 546 3515 Fax: 706 546 3068, e-mail: jarnold-at-ars.usda.gov. Completed nominations should be submitted before December 1, 2002.
Paula Allan-Wojtas, Chair, Food Structure and Functionality Forum - a division of AOCS.
Paula Allan-Wojtas Research Scientist - Food Microstructure Agriculture and Agri-Food Canada Atlantic Food and Horticulture Research Centre Kentville, Nova Scotia Canada B4N 1J5
I, too, would be interested in information on JEOL 2010F TEM's in the US.
Thanks to all,
Gary M. Brown ExxonMobil Chemical Company Baytown Polymers Center 5200 Bayway Drive Baytown, Texas 77520-2101 phone: (281) 834-2387 fax: (281) 834-2395 e-mail: Gary.M.Brown-at-ExxonMobil.com
No one said anything about "classified" data in this discussion other than to refer to who may have an interest in this. Technology such as data retrieval is practiced in numerous industries not the least of which is data comm.
Mr. Aschcroft may inspect my hard drive at his leisure.
Peter Tomic
-----Original Message----- } From: Michael Cammer [mailto:cammer-at-aecom.yu.edu] Sent: Sunday, September 22, 2002 9:36 PM To: Allen Sampson Cc: '"simkin-at-egr.msu.edu"-at-sparc5.microscopy.com'; Microscopy-at-sparc5.microscopy.com
If you pursue this discussion any further, I suspect you will have violated the new Patriot Act and numerous other laws forbidding discussion of the possibility of maybe uncovering classified data. -Michael
Please note that the date in the last sentence is incorrect. The nominations should be submitted by NOVEMBER 1, 2002. Thanks, Judy } } } "Paula Allan-Wojtas" {AllanWojtasP-at-agr.gc.ca} 09/23/02 08:51AM } } } CALL FOR NOMINATIONS FOOD STRUCTURE AND FUNCTIONALITY DIVISION ( at AOCS) AWARD
This award honors outstanding lifetime performance and meritorious contributions to an area of interest to the Food Structure & Functionality Division of the American Oil Chemists' Society. The award will be presented during the 94th AOCS annual Meeting & Exp to be held in Kansas City, Missouri, May 4-7, 2003 and consists of $1,500USD to help defray costs incurred by the awardee in participating in the AOCS Annual Meeting & Expo, and also a crystal plaque.
Nominations should consist of a letter of nomination, supporting letters from at least three other scientists, and biographical information concerning the nominee. The biographical information must include a summary of the nominee's research accomplishments, a list of publication, degree(s) held (with the names of granting institutions) and positions(s) held during the nominee's professional career.
For further information on nomination procedures contact the Food Structure & Functionality Division Award Canvassing Committee Chairperson, Dr, Judy Arnold, USDA-ARS_RRC, 950 College Station Rd., P.O. Box 5677, Athens, GA 30604-5677, USA, Tel: 706 546 3515 Fax: 706 546 3068, e-mail: jarnold-at-ars.usda.gov. Completed nominations should be submitted before December 1, 2002.
Paula Allan-Wojtas, Chair, Food Structure and Functionality Forum - a division of AOCS.
Paula Allan-Wojtas Research Scientist - Food Microstructure Agriculture and Agri-Food Canada Atlantic Food and Horticulture Research Centre Kentville, Nova Scotia Canada B4N 1J5
Tel: (902) 679-5566 FAX: (902) 679-2311
email: allanwojtasp-at-agr.gc.ca
______________________________ Judy W. Arnold, Ph.D. Research Microbiologist USDA-ARS, Russell Research Center 950 College Station Road Athens, GA 30605
Does anyone has experience embedding and polymerisation of Unicryl with Leica AFS? I am preparing sample for LM and EM immunolabeling. I embed sample with Unicryl and cure the resin in Leica AFS at 4C for more than 4 days. The resin still looks partially cured. I was wondering if it was UV intensity problem or other problem. Any suggestion and references are appreciated!!! Thanks.
Shanling
Shanling Shi Advanced Imaging & Measurement Unilever Research US 45 River Road Edgewater, NJ 07020 201-840-2340 Shanling.Shi-at-unilever.com
that is an interesting observation. which section of the patriot act are you speaking of and which other laws (new or old) might be involved? sterling
On Sun, 22 Sep 2002, Michael Cammer wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } If you pursue this discussion any further, I suspect you will have } violated the new Patriot Act and numerous other laws forbidding } discussion of the possibility of maybe uncovering classified data. } -Michael } }
} Email: spyker-at-bright.net } Name: lauren } } Organization: Perry Jr. High } } Education: 6-8th Grade Middle School } } Location: Lima, Ohio USA } } Question: What is the best way to prepare an insect wing for a slide mount... } } --------------------------------------------------------------------------- Lauren -
Let's keep this simple. To avoid damage, you should use a cover slip over the wing. You need some kind of a mounting medium under the coverslip. Water is OK for a temporary mount, but for permanance, use glycerin, clear nail polish, or "liquid bandage" from a drugstore. If you use glycerin, which never dries, you'll need to seal the coverslip edges with nailpolish. An entomologist in Texas uses a fascinating approach to low magnification study of dragonfly wings. He chills a live dragonfly in a refrigerator, places it in his computer scanner, and makes a hi-res scan. When it warms up, it can fly away. Directions and beautiful images are at http://stephenville.tamu.edu/~fmitchel/dragonfly/index.html
Caroline
Caroline Schooley Project MICRO Coordinator Microscopy Society of America Box 117, 45301 Caspar Point Road Caspar, CA 95420 Phone/FAX (707)964-9460 Project MICRO: http://www.msa.microscopy.com/ProjectMicro/PMHomePage.html Intertidal invertebrates: http://www.fortbragg.k12.ca.us/AG/marinelab.html
} From: "Dirk Kirch" {kirch-at-imm.rwth-aachen.de} To: Microscopy-at-sparc5.microscopy.com Date sent: Mon, 23 Sep 2002 10:51:37 +0200
Ok, I admit it was a bad joke. Apologies.
} } If you pursue this discussion any further, I suspect you will have } } violated the new Patriot Act and numerous other laws forbidding } } discussion of the possibility of maybe uncovering classified data. } } -Michael } } } }
dear listers, does anyone know the proper way to take the top off a reichert ultracut e ultramicrotome? tia, beth
********************************************************************** Beth Richardson EM Lab Coordinator Plant Biology Department University of Georgia Athens, GA 30602-7271
Phone - (706) 542-1790 & FAX - (706) 542-1805
"Between the two evils, I always pick the one I never tried before". Mae West (1893-1980) **********************************************************************
"And it's only the giving that makes you what you are". Wond'ring Aloud, Jethro Tull (Aqualung)
We have had a Nanoscope AFM since about 1994 and one of the features the students use in the software is the simple TIFF export function that converts just the image data to a grayscale (or color) TIFF image.
We recently upgraded the software on both of our AFM systems to version 5.12r3. The TIFF export menu is still there but it doesn¹t let you export just the image data, now you have to export the whole screen and then use another image processing program to extract just the image data! In the manual for this version it says that you can do just the image but there is no option for it in the software.
I called DI and asked about this and the tech support guy didn¹t know why it wasn't there and went to ask the programmers and here is the exact reply I got:
"As far as the Tiff export goes, I talked to some of our software guys. They tell me the File export for the TIFF never worked very well so they took it out. But, the file can be cropped in PhotoShop."
Well, we had been using it for nearly 8 years, but I guess we are no judges of how well it works! So they arbitrarily changed the functionality of the software and didn¹t even both to change the manual or tell anyone! They seem to be able to save the whole screen easily enough, but not the file data, how weird is that? Even I could program the saving of a simple TIFF file, but apparently this is beyond the software engineers at DI. I wrote back and asked for an explanation and was promptly ignored. So I thought this tirade to the net community might wake up someone at DI.
Just so you know, these are my opinions and thoughts, however unreasoanable, my employer has no connection to them whatsoever.
-- John Mansfield PhD MInstP North Campus Electron Microbeam Analysis Laboratory 417 SRB, University of Michigan 2455 Hayward, Ann Arbor MI 48109-2143 Phone: (734) 936-3352 FAX (734) 763-2282 Cell. Phone: (734) 834-3913 (Leaving a phone message at 936-3352 is preferable to 834-3913) Email: jfmjfm-at-engin.umich.edu URL: http://emalwww.engin.umich.edu/people/jfmjfm/jfmjfm.html Location: Lat. 42! 16' 48" Long. 83! 43' 48"
Graduate students wanted for Materials Sciences and TEM work
The Information Technology Initiative of Louisiana supplies a grant for graduate students to enter a 4 year PhD program at the University of New Orleans. Projects include characterization of transition metal oxides (crystallography, lattice defect analysis) and in-situ heating experiments of two phases alloys.
Contact :
Heike Gabrisch Assistant Professor of Chemistry and Material Sciences Department of Chemistry/AMRI University of New Orleans New Orleans, LA 70148
I'd be happy to join this tirade. I met John a few years ago at UM - between his rep in the field, his postings here and that meeting, I know him to be a force in microscopy. As a programmer, I also know how right he is in his outrage at such assertions from a manufacturer.
It's clear from what he is being told that the programmers at DI are simply doing a screen dump to TIFF, using the image data written to the screen object. This is unfortunate as the resolution will also be limited to that of the screen. The TIFF file structure was intentionally designed to be open and simple in order to be a widely used standard. A directory contains the location of file elements, a number of 'tags' are written that describe the file contents and the data is written to the file in a simple format.
Ideally, when writing a TIFF file from a program like this, all acquired data will be written to the file as a graphical representation that uses the same resolution and data as that of the original scans. Programs used later in the presentation can then adjust the image for whatever needs you may have. The TIFF standards allow for easy methods to write this data to file in a way that can be understood by any programs that also follow TIFF standards. In our work, TIFF is severely limited in several ways, but is currently the best method to transfer image data.
Scanning probe methods create data that is not generally depicted as it is. The Z axis data, or intensity of a two dimensional image, is normally translated, as well as the X and Y data, into a rotationally translated image representing surface topography. Thus the data collected needs this imaging translation for presentation.
Windows gives you various canvasses to draw image data on - the screen and printer are two better known examples. When drawing to any of these canvases, the first job is to determine their capabilities, i.e. resolution, and adjust your drawing to those limitations. But you can also create 'phantom' canvases that have arbitrary resolutions. These are basically memory spaces that the image data is written to. Once they are completed, you have a set of data that is appropriate for directly exporting to TIFF format. This background operation can be completed in a fraction of a second and a TIFF file created in a second or two, depending on the size.
I hope this gives enough of a hint to the DI programmers on how to do it, if not please feel free fire their asses or have them contact me. This is an egregious situation for a company who's livelihood relies on computers.
Just so you know, these are my own opinions and thoughts, and I am my own employer. I always call it like I see it, and what I see here stinks.
Allen R. Sampson Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174
On Monday, September 23, 2002 12:51 PM, John Mansfield [SMTP:jfmjfm-at-umic h.edu] wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } We have had a Nanoscope AFM since about 1994 and one of the features the } students use in the software is the simple TIFF export function that } converts just the image data to a grayscale (or color) TIFF image. } } We recently upgraded the software on both of our AFM systems to version } 5.12r3. The TIFF export menu is still there but it doesn?t let you export } just the image data, now you have to export the whole screen and then use } another image processing program to extract just the image data! In the } manual for this version it says that you can do just the image but there is } no option for it in the software. } } I called DI and asked about this and the tech support guy didn?t know why it } wasn't there and went to ask the programmers and here is the exact reply I } got: } } "As far as the Tiff export goes, I talked to some of our software guys. They } tell me the File export for the TIFF never worked very well so they took it } out. But, the file can be cropped in PhotoShop." } } Well, we had been using it for nearly 8 years, but I guess we are no judges } of how well it works! So they arbitrarily changed the functionality of the } software and didn?t even both to change the manual or tell anyone! They } seem to be able to save the whole screen easily enough, but not the file } data, how weird is that? } Even I could program the saving of a simple TIFF file, but apparently this } is beyond the software engineers at DI. I wrote back and asked for an } explanation and was promptly ignored. So I thought this tirade to the net } community might wake up someone at DI. } } Just so you know, these are my opinions and thoughts, however unreasoanable, } my employer has no connection to them whatsoever. } } } -- } John Mansfield PhD MInstP } North Campus Electron Microbeam Analysis Laboratory } 417 SRB, University of Michigan } 2455 Hayward, Ann Arbor MI 48109-2143 } Phone: (734) 936-3352 FAX (734) 763-2282 Cell. Phone: (734) 834-3913 } (Leaving a phone message at 936-3352 is preferable to 834-3913) } Email: jfmjfm-at-engin.umich.edu } URL: http://emalwww.engin.umich.edu/people/jfmjfm/jfmjfm.html } Location: Lat. 42! 16' 48" Long. 83! 43' 48" } } } } }
The rule of Law should be that if you start to read someone's hard drive, you must do it bit-by-bit until you are bitten through!
Assuming that I understand the original question, which I now can't remember - half the fun - here's a real look at data conservation by those who will, in the end, have to be prepared for it, the Archaeologists.
Fred Monson Frederick C. Monson, PhD Center for Advanced Scientific Imaging Geology-Astronomy West Chester University of Pennsylvania Schmucker Science Center II South Church street & Rosedale Avenue West Chester, PA, 19383, USA Phone: 610-738-0437 FAX: 610-738-0437 eMail: fmonson-at-wcupa.edu http://darwin.wcupa.edu/casi/ http://www.wcupa.edu/_visitors/
-----Original Message----- } From: Peter Tomic [mailto:PTomic-at-anadigics.com] Sent: Monday, September 23, 2002 9:56 AM To: 'Michael Cammer'; Allen Sampson Cc: '"simkin-at-egr.msu.edu"-at-sparc5.microscopy.com'; Microscopy-at-sparc5.microscopy.com
No one said anything about "classified" data in this discussion other than to refer to who may have an interest in this. Technology such as data retrieval is practiced in numerous industries not the least of which is data comm.
Mr. Aschcroft may inspect my hard drive at his leisure.
Peter Tomic
-----Original Message----- } From: Michael Cammer [mailto:cammer-at-aecom.yu.edu] Sent: Sunday, September 22, 2002 9:36 PM To: Allen Sampson Cc: '"simkin-at-egr.msu.edu"-at-sparc5.microscopy.com'; Microscopy-at-sparc5.microscopy.com
If you pursue this discussion any further, I suspect you will have violated the new Patriot Act and numerous other laws forbidding discussion of the possibility of maybe uncovering classified data. -Michael
The Department of Materials Science and Metallurgy at Cambridge has a world-class suite of fifteen electron microscopes, both transmission and scanning, and four electron microscope technicians.
Applications are invited for a Senior Technical Officer who will ensure that the microscopes operate at peak performance and who will be responsible for training users, both from within Cambridge University and from outside, and interacting with microscope manufacturers. The post holder will have a detailed knowledge of electron optics, vacuum systems, etc., a background in physical science, and will be an expert user of electron microscopes and their analytical attachments. It is not essential, but it would be an advantage, if the person appointed could also give graduate lectures in electron microscopy, be knowledgeable about image simulation software and computing, develop new electron microscope techniques and engage in research. However, the post is essentially a very high level research support position.
This is a permanent position funded by the University of Cambridge. The initial appointment will be for a period of five years, which may be renewed until retirement. Salary will be in the range £22,522 to £32,537.
Further information about this position may be obtained by contacting
Dr Paul Midgley, Tel. +44 (0)1223 334561, E-mail: pam33-at-cam.ac.uk or Professor Colin Humphreys, Tel. +44 (0)1223 334457, E-mail: colin.humphreys-at-msm.cam.ac.uk.
Applications, which should be in writing and include a CV and the names and addresses of three referees, should be sent to:
Ms Lorraine Dann, Departmental Administrator, Department of Materials Science and Metallurgy, University of Cambridge, Pembroke Street, Cambridge, CB2 3QZ, UK.
Dear all, I am wanting to do image simulation of HREM images from a JEOL 3010 (LaB6 filament). Does anyone know the spread of defocus due to chromatic abberation for this microscope?
Also, I need to determine the semiangle of beam convergence. I assume I just do this by photographing a convergent beam diffraction pattern made using the same condensor aperture as for the image and calculating the angle from the diffraction disk radius. Am I right?
Best wishes
-- Ian MacLaren Strukturforschung, Materialwissenschaft, TU-Darmstadt, Germany ian.maclaren-at-physics.org / http://homepages.tu-darmstadt.de/~maclaren/
To remove the cover of an Ultracut E, there are a few things you must do.
1) Turn the stage course wheel located at the front of the machine counter clockwise to move the stage towards you.
2) The remove the 2 large flat head screws located on the plate that surrounds the stage. There will be on screw on each side. Completely remove them.
3) Remove this plate but lifting it up and around the knife stage.
4) By removing that plate, it now makes visible two allen screws located on each side of the microtome. The screws go through a bracket that holds down the front of the cover. Completely remove these two screws, and remove the brackets.
5) Lastly, you must remove the two allen key screws located at the rear of the instrument towards the bottom on the backside of the cover. One these are removed you are ready to remove the cover.
Things to check before removing the cover are: Specimen arc and chuck should be removed Spring loaded set screw that hold the specimen arc in place should be removed completely Handwheel needs to be removed (1 allen key screw located at the center of the handwheel) Remove knife holder from stage
Once all these steps are followed you should be able to remove the cover completely. When placing the cover back onto the instrument, please be sure to observe the serial port connection located at the back of the unit. The male end of this plug is located on the cover and the female end is located on the back portion of the microtome. You must be sure that when placing the cover back on, that these two connections are plugged into each other in order for the microtome to operate.
If you have any questions, please feel free to contact Leica's TAC Center at 1-800-248-0123 Option 3, then Option 1.
Best Regards, Shawn LaRocco Manager, Service Administration and TAC 847.317.7263
Apparently part of the "microscopy-at-sparc5.microscopy.com" was missing.
What can I do for you?
Gary M. Brown ExxonMobil Chemical Company Baytown Polymers Center 5200 Bayway Drive Baytown, Texas 77520-2101 phone: (281) 834-2387 fax: (281) 834-2395 e-mail: Gary.M.Brown-at-ExxonMobil.com
"Bob Roberts" {bobrobs-at-cox.ne To: {Gary.M.Brown-at-ExxonMobil.com} t} cc: Subject: Recent Reply to Listserver Message
09/23/02 08:29 PM
Hi Gary,
I just sent you a reply and it was addressed kinda weird. It had your above email address but with "-at-sparc5microscopy.com" added to the end. Not sure about how this happened. Any way if you didn't receive it, please let me know.
Bob Roberts EM Lab Services, Inc. 449 NW 62nd St Topeka, Kansas 66617-1780 785.246.1232 www.emlabservices.com
Beth, Look where the head is attached to the body, you will see a screw with one flat side, turn that until the head can be slid off with the back/foward knob. That should do it (you may have to turn the head to the left). Mike D
Beth Richardson wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } dear listers, } does anyone know the proper way to take the top off a reichert ultracut e } ultramicrotome? } tia, } beth } } ********************************************************************** } Beth Richardson } EM Lab Coordinator } Plant Biology Department } University of Georgia } Athens, GA 30602-7271 } } Phone - (706) 542-1790 & FAX - (706) 542-1805 } } "Between the two evils, } I always pick the one I never tried before". Mae West (1893-1980) } ********************************************************************** } } "And it's only the giving that makes you what you are". } Wond'ring Aloud, Jethro Tull (Aqualung) } } ***************************************************************************
Remove knife block and specimen block. Back up the top piece with binoculars are far as it will go - you need to gently push on it as you turn the knob. As it moves back, you can see the plug where the upper lamp is plugged in. Unplug this, and continue backing up the top until it comes off. Place it somewhere safe - don't let the eyepieces fall out! You can remove the whole binoc assembly first if you are worried.
Remove the metal rim that runs around the knife block. there are two slotted screws at the rear of the plate - just in front of where the holes for the little specimen key lives. Lift off the plate by gently tilting the plate forward to get it off around the little lever in front that locks the knife block in place.
once that plate is removed, you can see two L-shaped brackets that are held down by allen screws that hold the front end of the top in place. remove them.
Next remove the two allen screws at the back of the microtome near the bottom of the top cover. You can now remove the top by gently lifting up. Next, gasp at all the crud that has built up inside! I have done this a bunch of times without a problem. Keyword = GENTLE. Good luck, tom
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
-- Thomas E. Phillips, Ph.D. Associate Professor of Biological Sciences Director, Molecular Cytology Core Facility
3 Tucker Hall Division of Biological Sciences University of Missouri Columbia, MO 65211-7400 (573)-882-4712 (voice) (573)-882-0123 (fax)
Thanks for all the emails and phone calls about taking the top off the Reichert! I have the information that I need now. This list is the best! thanks again, Beth
********************************************************************** Beth Richardson EM Lab Coordinator Plant Biology Department University of Georgia Athens, GA 30602-7271
Phone - (706) 542-1790 & FAX - (706) 542-1805
"Between the two evils, I always pick the one I never tried before". Mae West (1893-1980) **********************************************************************
"And it's only the giving that makes you what you are". Wond'ring Aloud, Jethro Tull (Aqualung)
I have been having trouble collecting film based elemental X-ray maps on my Jeol 733 at a magnification of 40X. The map of a mineral grain that fills the screen at this mag (2.5mmx2.5mm?) only shows a concentration of dots diagonally near the center of the grain. I suspect I may be beyond the area in which I can collect X-rays or someting is misaligned. Any comments will be appreciated.
Thanks
Roy Beavers Southern Methodist University Department of Geological Sciences P.O. Box 750395 Dallas, Tx. 75275 Voice: 214-768-2756 Fax: 214-768-2701 Email: rbeavers-at-mail.smu.edu
The spec. for the JEOL 3010 gives Cc as polepiece dependent. The UHR polepiece has Cc=1.3 mm and the HR has 1.8 mm.
The defocus spread is given as Cc*(delta(E)/E), roughly, where delta(E) is the energy spread of the source. This assumes that the contribution due to objective lens current fluctuation is negligible (see for example O. Krivanek "Practical High Resolution Electron Microscopy" in a book edited by Buseck et al, 1984 (Oxford)). Now delta(E) is dependent on how you run your filament, but might be somewhere in the range of a couple of eV for a thermionic gun. So a good estimate of defocus spread would be somewhere about 100 Angstroms. I would be interested if anyone can provide a more accurate value than this, or if I am seriously off here.
On the second point: You cannot always simply go to crossover and measure the radius of your CBED disks in order to get the beam convergence for estimating spatial coherence. Specifically, if you are doing HREM imaging with a defocused beam on your sample, the act of defocusing is actually increasing coherence locally. The angular spread of the beam at a single point is a lot less than the total spread across the whole illuminated area. On older TEM's one typically operated close to crossover (filament image on sample, and angular spread at a point in the back focal plane) so it was possible to use the diffraction pattern to estimate spatial coherence, as described by a 1975 article by O'Keefe and Sanders (in Acta Cryst.). If on the other hand you're operating with a spread beam you will see small bright and dark field images in the BFP. Since you are imaging angles in the BFP the occurrence of images is just saying that the incident angle varies across the illuminated area. The coherence is determined by the uncertainty in the angle at a single point in your HREM image.
So how do you measure convergence if you are not recording images at crossover? Maybe you can decrease your condenser aperture as small as you can go and still get comparable intensity, then measure the angular spread in the BFP. Another approach might be to set up the conditions used for imaging, then go to diffraction mode and re-focus the diffraction pattern (decrease the intermediate lens current) to obtain sharp filament images, then measure the half-width of the filament images relative to the absolute scaling provided by the pattern. This will at any rate be better than using the total angular range within the condenser aperture.
Regards,
Wharton Sinkler UOP LLC Des Plaines, IL 60017-5017 U. S. A.
} -----Original Message----- } From: Ian MacLaren [SMTP:maclaren-at-tu-darmstadt.de] } Sent: Tuesday, September 24, 2002 7:22 AM } To: Microscopy } Subject: HREM simulation / JEOL 3010 } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Dear all, } I am wanting to do image simulation of HREM images from a JEOL 3010 } (LaB6 filament). Does anyone know the spread of defocus due to } chromatic abberation for this microscope? } } Also, I need to determine the semiangle of beam convergence. I assume } I just do this by photographing a convergent beam diffraction pattern } made using the same condensor aperture as for the image and calculating } the angle from the diffraction disk radius. Am I right? } } Best wishes } } -- } Ian MacLaren } Strukturforschung, Materialwissenschaft, TU-Darmstadt, Germany } ian.maclaren-at-physics.org / http://homepages.tu-darmstadt.de/~maclaren/ }
I missed MSA this year (fell off my bike, broke some things) so I didn't get a chance to catch up on the latest and greatest regarding the current state of the art for printing digital images etc.
Here's my dilema: We have a fancy dye sub printer, but it just broke and needs repair. We have had it since 1996 and it got lots of use in the first 4 or 5 years, but business has fallen off lately, like down to one or two uses in the last several months. I am trying to figure out what is happening, my guess is that everyone is using some cheap new ink jets in their own lab to do their printing. We are a small central services type lab, our users visit us to use the instruments, then take their image files with them. The dye sub used to get a lot of use from all kinds of people on campus, but no longer.
So, what's up with printing? Do I get the dye sub fixed, or do I save the $$ and buy a couple of photo ink jet things to do its job? There has been a major transformation in imaging technologies here, our darkroom is practically abandoned, the dye sub is mostly idle etc. Has printing become a distributed resource where everyone does it independently, or have some just given up on printing altogether and everything gets distributed and submitted in electronic form?
Just curious.
Jonathan Krupp Microscopy & Imaging Lab University of California Santa Cruz, CA 95064 (831) 459-2477 jmkrupp-at-cats.ucsc.edu
I was totally with you right up until the point you chose to use vulgarity, thereby losing any respect I had for your argument. It did not make you look very professional, but of course, this is also my own opinion and does not reflect that of my company. I will not comment further on this thread other than to say that I, too, think DI could do a better job of the tiff export function, especially where image analysis may be performed on the images post export.
Sincerely,
David Bell Scientist Electron Microscopy Lab Millipore Corporation 80 Ashby Road Bedford, MA 01730 (781) 533-2108
Allen Sampson {ars-at-sem.com} 09/24/2002 03:43 AM Please respond to "ars-at-sem.com"
To: "'John Mansfield'" {jfmjfm-at-umich.edu} , "microscopy-at-microscopy.com" {microscopy-at-microscopy.com} cc: Subject: RE: DI AFM Software missing TIFF Export
------------------------------------------------------------------------ The Microscopy ListServer -- Sponsor: The Microscopy Society of America
I'd be happy to join this tirade. I met John a few years ago at UM - between his rep in the field, his postings here and that meeting, I know him to be a force in microscopy. As a programmer, I also know how right he is in his outrage at such assertions from a manufacturer.
It's clear from what he is being told that the programmers at DI are simply doing a screen dump to TIFF, using the image data written to the screen object. This is unfortunate as the resolution will also be limited to that of the screen. The TIFF file structure was intentionally designed to be open and simple in order to be a widely used standard. A directory contains the location of file elements, a number of 'tags' are written that describe the file contents and the data is written to the file in a simple
format.
Ideally, when writing a TIFF file from a program like this, all acquired data will be written to the file as a graphical representation that uses the same resolution and data as that of the original scans. Programs used
later in the presentation can then adjust the image for whatever needs you
may have. The TIFF standards allow for easy methods to write this data to
file in a way that can be understood by any programs that also follow TIFF
standards. In our work, TIFF is severely limited in several ways, but is currently the best method to transfer image data.
Scanning probe methods create data that is not generally depicted as it is. The Z axis data, or intensity of a two dimensional image, is normally translated, as well as the X and Y data, into a rotationally translated image representing surface topography. Thus the data collected needs this
imaging translation for presentation.
Windows gives you various canvasses to draw image data on - the screen and
printer are two better known examples. When drawing to any of these canvases, the first job is to determine their capabilities, i.e. resolution, and adjust your drawing to those limitations. But you can also create 'phantom' canvases that have arbitrary resolutions. These are basically memory spaces that the image data is written to. Once they are completed, you have a set of data that is appropriate for directly exporting to TIFF format. This background operation can be completed in a
fraction of a second and a TIFF file created in a second or two, depending
on the size.
I hope this gives enough of a hint to the DI programmers on how to do it, if not please feel free fire their asses or have them contact me. This is
an egregious situation for a company who's livelihood relies on computers.
Just so you know, these are my own opinions and thoughts, and I am my own employer. I always call it like I see it, and what I see here stinks.
Allen R. Sampson Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174
On Monday, September 23, 2002 12:51 PM, John Mansfield [SMTP:jfmjfm-at-umic h.edu] wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } We have had a Nanoscope AFM since about 1994 and one of the features the } students use in the software is the simple TIFF export function that } converts just the image data to a grayscale (or color) TIFF image. } } We recently upgraded the software on both of our AFM systems to version } 5.12r3. The TIFF export menu is still there but it doesn?t let you export } just the image data, now you have to export the whole screen and then use } another image processing program to extract just the image data! In the } manual for this version it says that you can do just the image but there
is } no option for it in the software. } } I called DI and asked about this and the tech support guy didn?t know why it } wasn't there and went to ask the programmers and here is the exact reply
I } got: } } "As far as the Tiff export goes, I talked to some of our software guys. They } tell me the File export for the TIFF never worked very well so they took
it } out. But, the file can be cropped in PhotoShop." } } Well, we had been using it for nearly 8 years, but I guess we are no judges } of how well it works! So they arbitrarily changed the functionality of the } software and didn?t even both to change the manual or tell anyone! They } seem to be able to save the whole screen easily enough, but not the file } data, how weird is that? } Even I could program the saving of a simple TIFF file, but apparently this } is beyond the software engineers at DI. I wrote back and asked for an } explanation and was promptly ignored. So I thought this tirade to the net } community might wake up someone at DI. } } Just so you know, these are my opinions and thoughts, however unreasoanable, } my employer has no connection to them whatsoever. } } } -- } John Mansfield PhD MInstP } North Campus Electron Microbeam Analysis Laboratory } 417 SRB, University of Michigan } 2455 Hayward, Ann Arbor MI 48109-2143 } Phone: (734) 936-3352 FAX (734) 763-2282 Cell. Phone: (734) 834-3913 } (Leaving a phone message at 936-3352 is preferable to 834-3913) } Email: jfmjfm-at-engin.umich.edu } URL: http://emalwww.engin.umich.edu/people/jfmjfm/jfmjfm.html } Location: Lat. 42! 16' 48" Long. 83! 43' 48" } } } } }
In reference to printers, we are a university core facility and serve a broad spectrum of student and faculty users from 45 different departments. We have laser jet, ink jet, dye sub, and silver halide digital printers. The dye sub has received less and less use as the years have gone by. It is a Tektronix Phaser 440 which at one time was the work horse of the graphic arts industry. However, Tektronix completely dropped out of the dye sub market over a year ago. In fact, we can no longer buy supplies for it.
Most students now incorporate images directly into thesis text and print on a laser jet or ink jet printer. More and more journals are accepting and even preferring electronic submission. However, there are a substantial number of users and journals that insist on photographic quality output. These users have switched to our silver halide digital printer, a Fuji Pictrography 3000. The output from this is a photo in the true sense of the word because it uses silver halide technology similar to a photograph. In my opinion, it is far better than we ever got from the dye sub printer. Many professional photo labs are buying these for users that want the best possible output.
This has been our experience. Hope it helps.
Stanley L. Flegler, Director Center for Advanced Microscopy Michigan State University
I think I would concur with your guesses. Everyone is probably doing it on their own.
Current inkjet printers CAN do a quite good job rendering images on good paper. I have heard John Mc Kenzie recommend them at his seminars. Granted that many inkjets are still slow compared to other technologies. John even suggests setting up a bank of relatively cheap inkjets to share the jobs and keep through-put up. We haven't gone that route yet.
Users may also be settling for mediocre prints from their own printers not knowing what quality is available. We have an aging Lexmark Optra Rt+ that does a quite good job of printing B/W images on bright white paper. I just passed some prints from it on to a user who had tried printing images on his own printer. He much preferred our quality once he saw the prints. He just assumed, falsely in this case, that he could get the same quality on his own. Maybe you should post a classic image next to your printer so your users see what you can do.
But having said that, I probably would consider retiring the printer depending on the cost of repair. Printer technology has come a long way in recent years and the new stuff generally does better for cheaper.
Warren
At 10:03 AM 9/24/02 -0700, you wrote:
} Hi: } } I missed MSA this year (fell off my bike, broke some things) so I didn't } get a chance to catch up on the latest and greatest regarding the current } state of the art for printing digital images etc. } } Here's my dilema: We have a fancy dye sub printer, but it just broke and } needs repair. We have had it since 1996 and it got lots of use in the first } 4 or 5 years, but business has fallen off lately, like down to one or two } uses in the last several months. I am trying to figure out what is } happening, my guess is that everyone is using some cheap new ink jets in } their own lab to do their printing. We are a small central services type } lab, our users visit us to use the instruments, then take their image files } with them. The dye sub used to get a lot of use from all kinds of people on } campus, but no longer. } } So, what's up with printing? Do I get the dye sub fixed, or do I save the } $$ and buy a couple of photo ink jet things to do its job? There has been a } major transformation in imaging technologies here, our darkroom is } practically abandoned, the dye sub is mostly idle etc. Has printing become } a distributed resource where everyone does it independently, or have some } just given up on printing altogether and everything gets distributed and } submitted in electronic form? } } Just curious. } } Jonathan Krupp } Microscopy & Imaging Lab } University of California } Santa Cruz, CA 95064 } (831) 459-2477 } jmkrupp-at-cats.ucsc.edu
------------------------------------------- No files should be attached to this message ------------------------------------------- Warren E. Straszheim, Ph.D. Materials Analysis and Research Lab Iowa State University 23 Town Engineering Ames IA, 50011-3232
It sure sounds like you are seeing the effect of the alignment of your spectrometer. We used to have a WDS system on our SEM. We posted a couple of images comparing WDS and EDS x-ray maps next to our scope. Two things were quite apparent.
First, the better P/B ratio of WDS led to very low backgrounds and much better contrast in the WDS maps compared to the EDS maps. Second, we saw the intensity fall-off to the sides of the low-mag WDS maps due to misalignment. The spectrometer was simply optimized for measuring intensities at the center of the screen. By the time you moved the beam a millimeter or two to the edge of the area, you screwed up your diffraction conditions. We got a band of intensity that plainly showed us the position of the spectrometer with respect to the raster and also the alignment of the spectrometer (inclined or vertical).
You should be able to tweak your spectrometer settings by opening up the slits, if I recall correctly, to reduce this effect. However, it will probably still show more fall-off in intensity than does the EDS map.
Warren
At 10:49 AM 9/24/02 -0500, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
------------------------------------------- No files should be attached to this message ------------------------------------------- Warren E. Straszheim, Ph.D. Materials Analysis and Research Lab Iowa State University 23 Town Engineering Ames IA, 50011-3232
Roy- What you are seeing in the Rowland Circle.... That is, the only part of the beam raster that falls on the Rowland circle such that x-rays will be diffracted. No amount of 'tweeking' will allow you to fill the screen with x-rays at 40x if you are using WDS. For WDS x-ray maps the beam raster must fall completely on the Rowland circle so magnifications of greater then something like 1000x are needed. EDS can be used at low mags as there is no Rowland circle requirement, though I always collect EDS maps at the spectrometer focus (ie, sample is focused to the crosshairs in reflected light). scott
************************************************ ....amphiboles do violence to history... T. Feininger, 2001. (taken out of context) ****************************
Dr. Scott Kuehner kuehner-at-u.washington.edu Dept. of Geological Sciences ph.206-543-8393 Box 351310 Fax 206-616-6873 The University of Washington Seattle, Washington 98195-1310 ************************************************
On Tue, 24 Sep 2002, Beavers, Roy wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Group } } I have been having trouble collecting film based elemental X-ray maps on my Jeol 733 at a magnification of 40X. The map of a mineral grain that fills the screen at this mag (2.5mmx2.5mm?) only shows a concentration of dots diagonally near the center of the grain. I suspect I may be beyond the area in which I can collect X-rays or someting is misaligned. Any comments will be appreciated. } } Thanks } } Roy Beavers } Southern Methodist University } Department of Geological Sciences } P.O. Box 750395 } Dallas, Tx. 75275 } Voice: 214-768-2756 } Fax: 214-768-2701 } Email: rbeavers-at-mail.smu.edu } } }
Measure the time it takes to print an image of a Codonics 1600 (if you can get it to work) and then measure the time it takes to print an image on an Epson 980 or similar (the one's we happen to use) and then look at the cost difference and see that I'd go for the Epson anytime. They're disposable.
Again, MY opinion, no one else's!
On 9/24/02 2:23 PM, "Warren E Straszheim" {wesaia-at-iastate.edu} wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } I think I would concur with your guesses. Everyone is probably doing it on } their own. } } Current inkjet printers CAN do a quite good job rendering images on good } paper. I have heard John Mc Kenzie recommend them at his seminars. Granted } that many inkjets are still slow compared to other technologies. John even } suggests setting up a bank of relatively cheap inkjets to share the jobs } and keep through-put up. We haven't gone that route yet. } } Users may also be settling for mediocre prints from their own printers not } knowing what quality is available. We have an aging Lexmark Optra Rt+ that } does a quite good job of printing B/W images on bright white paper. I just } passed some prints from it on to a user who had tried printing images on } his own printer. He much preferred our quality once he saw the prints. He } just assumed, falsely in this case, that he could get the same quality on } his own. Maybe you should post a classic image next to your printer so your } users see what you can do. } } But having said that, I probably would consider retiring the printer } depending on the cost of repair. Printer technology has come a long way in } recent years and the new stuff generally does better for cheaper. } } Warren } } At 10:03 AM 9/24/02 -0700, you wrote: } } } Hi: } } } } I missed MSA this year (fell off my bike, broke some things) so I didn't } } get a chance to catch up on the latest and greatest regarding the current } } state of the art for printing digital images etc. } } } } Here's my dilema: We have a fancy dye sub printer, but it just broke and } } needs repair. We have had it since 1996 and it got lots of use in the first } } 4 or 5 years, but business has fallen off lately, like down to one or two } } uses in the last several months. I am trying to figure out what is } } happening, my guess is that everyone is using some cheap new ink jets in } } their own lab to do their printing. We are a small central services type } } lab, our users visit us to use the instruments, then take their image files } } with them. The dye sub used to get a lot of use from all kinds of people on } } campus, but no longer. } } } } So, what's up with printing? Do I get the dye sub fixed, or do I save the } } $$ and buy a couple of photo ink jet things to do its job? There has been a } } major transformation in imaging technologies here, our darkroom is } } practically abandoned, the dye sub is mostly idle etc. Has printing become } } a distributed resource where everyone does it independently, or have some } } just given up on printing altogether and everything gets distributed and } } submitted in electronic form? } } } } Just curious. } } } } Jonathan Krupp } } Microscopy & Imaging Lab } } University of California } } Santa Cruz, CA 95064 } } (831) 459-2477 } } jmkrupp-at-cats.ucsc.edu } } ------------------------------------------- } No files should be attached to this message } ------------------------------------------- } Warren E. Straszheim, Ph.D. } Materials Analysis and Research Lab } Iowa State University } 23 Town Engineering } Ames IA, 50011-3232 } } Ph: 515-294-8187 } FAX: 515-294-4563 } } E-Mail: wesaia-at-iastate.edu } Web: www.marl.iastate.edu } } Scanning electron microscopy, x-ray analysis, and image analysis of materials } Computer applications and networking } } } }
-- John Mansfield PhD MInstP North Campus Electron Microbeam Analysis Laboratory 417 SRB, University of Michigan 2455 Hayward, Ann Arbor MI 48109-2143 Phone: (734) 936-3352 FAX (734) 763-2282 Cell. Phone: (734) 834-3913 (Leaving a phone message at 936-3352 is preferable to 834-3913) Email: jfmjfm-at-engin.umich.edu URL: http://emalwww.engin.umich.edu/people/jfmjfm/jfmjfm.html Location: Lat. 42! 16' 48" Long. 83! 43' 48"
Jonathan, Sorry about your bike encounter. Hope you're on the mend. I'm sure you'll get lots of responses re your printer query. We are also a central facility and also had a very expensive Kodak dye-sub that cost a fortune to repair. After the second breakdown, we spent the money on an Olympus dye-sub which is very nice and cost around $700. The only problem is that it will print only 3 colors, unlike the Kodak which had interchangeable ribbons for 4 color, 3 color, or black. The other printer we have which was even less expensive is an Epson photo stylus which prints nice images but they will fade in time. It is of course an ink jet and I buy good paper, but they still fade. They are inexpensive and a good source for "study prints" however. I think a lot of users copy to a CD and print in their own labs as we too have had a drop off in the printing business. Out of an average of 40 users a month, I have only one who still uses the darkroom. Good luck with your printer decision. Mary Gail Engle
At 10:03 AM 9/24/02 -0700, Jon Krupp wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Mary Gail Engle Sr. Research Laboratory Manager Electron Microscopy & Imaging Facility Health Sciences Research Bldg. 001 University of Kentucky Lexington, KY 40536-0305
Sounds to me like your detector is probably not fully looking at the area of sample you want to collect dot maps from. You probably have a collimator in the nose of your x-ray detector which limits field of view.
Usually, just need to adjust working distance, perhaps sample tilt also - toward detector - to bring area of interest onto axis, or line-of-sight, of detector. Put in a clean aluminum stub, turn up mag to a few hundred times, look at Al Ka x-rays count rate, and adjust working distance (keep image in focus) until you see maximum count rate. then you have sample area dead center on the axis of the EDS detector.
Also, because you are working at fairly low mag, only 40X, you may get some collimator clipping anyway, but if axis is aligned as above, it should just clip around the edges, circular-wise, like looking through a round hole.
For example, on my Hitachi S3500N, I need working distance of 16 mm (+ or - 1 mm) for optimum collection of x-rays.
Hope this helps!
Gib
Gib Ahlstrand Electron Optical Facility, University of Minnesota, CBS Imaging Center, 35 Snyder Hall, St. Paul, MN. USA. 55108 (612)624-3454 (612)625-5754 FAX, ahlst007-at-tc.umn.edu http://www.cbs.umn.edu/ic/
"You can learn a lot by observation - just by lookin'!" - Yogi Bera
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Group } } I have been having trouble collecting film based elemental X-ray maps on my } Jeol 733 at a magnification of 40X. The map of a mineral grain that fills the } screen at this mag (2.5mmx2.5mm?) only shows a concentration of dots } diagonally near the center of the grain. I suspect I may be beyond the area in } which I can collect X-rays or someting is misaligned. Any comments will be } appreciated. } } Thanks } } Roy Beavers } Southern Methodist University } Department of Geological Sciences } P.O. Box 750395 } Dallas, Tx. 75275 } Voice: 214-768-2756 } Fax: 214-768-2701 } Email: rbeavers-at-mail.smu.edu } } }
Dye sub is pretty much out except for Kodak PS86xx. But each print is rather pricey. Between the paper and the film, I figure that each 8.5x11 print costs about $1.50.
Epson has mostly replaced dye sub with their photo ink jets. Narrow size is the 890P and wide is the 9000P. They also make a super wide (36" or so wide, virtually infinite length). The quality on photo grade paper is awesome. But the speed of printing is depressing. Be prepared to wait with a six pack of your favorite beverage while printing an 11x17" print. But the results are very good.
Tonal range is good. Durability of the print is good. Cost of paper is good. The only down side is that the Epson photo ink jets use a CMYK ink cartridge system and are very proprietary (not refillable).... a tad pricey.
gary g.
At 10:03 AM 9/24/2002, you wrote:
} Hi: } } I missed MSA this year (fell off my bike, broke some things) so I didn't } get a chance to catch up on the latest and greatest regarding the current } state of the art for printing digital images etc. } } Here's my dilema: We have a fancy dye sub printer, but it just broke and } needs repair. We have had it since 1996 and it got lots of use in the first } 4 or 5 years, but business has fallen off lately, like down to one or two } uses in the last several months. I am trying to figure out what is } happening, my guess is that everyone is using some cheap new ink jets in } their own lab to do their printing. We are a small central services type } lab, our users visit us to use the instruments, then take their image files } with them. The dye sub used to get a lot of use from all kinds of people on } campus, but no longer. } } So, what's up with printing? Do I get the dye sub fixed, or do I save the } $$ and buy a couple of photo ink jet things to do its job? There has been a } major transformation in imaging technologies here, our darkroom is } practically abandoned, the dye sub is mostly idle etc. Has printing become } a distributed resource where everyone does it independently, or have some } just given up on printing altogether and everything gets distributed and } submitted in electronic form? } } Just curious. } } Jonathan Krupp } Microscopy & Imaging Lab } University of California } Santa Cruz, CA 95064 } (831) 459-2477 } jmkrupp-at-cats.ucsc.edu
It was late and it really grates when a good and innovative company begins down this path. The vulgarity wasn't necessary or warranted. This is also not a forum for the discussion of what, exactly, can be considered vulgarity in this day and age.
My most humble apologies to any and all who may have taken offense at my use of that one word. I promise to attempt to expand my meager vocabulary in other directions in the future. I'm sorry if that word detracted in any way from the other 493 I wrote.
Allen R. Sampson Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174
On Tuesday, September 24, 2002 10:22 AM, "David_Bell-at-millipore.com"-at-sparc5.microscopy.com [SMTP:"David_Bell-at-millipore.com"-at-sparc5.microscopy.com] wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Allen, } } I was totally with you right up until the point you chose to use } vulgarity, thereby losing any respect I had for your argument. It did not } make you look very professional, but of course, this is also my own } opinion and does not reflect that of my company. I will not comment } further on this thread other than to say that I, too, think DI could do a } better job of the tiff export function, especially where image analysis } may be performed on the images post export. } } Sincerely, } } } David Bell } Scientist } Electron Microscopy Lab } Millipore Corporation } 80 Ashby Road } Bedford, MA 01730 } (781) 533-2108 } } } } } } } Allen Sampson {ars-at-sem.com} } 09/24/2002 03:43 AM } Please respond to "ars-at-sem.com" } } } To: "'John Mansfield'" {jfmjfm-at-umich.edu} , "microscopy-at-microscopy.com" } {microscopy-at-microscopy.com} } cc: } Subject: RE: DI AFM Software missing TIFF Export } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } I'd be happy to join this tirade. I met John a few years ago at UM - } between his rep in the field, his postings here and that meeting, I know } him to be a force in microscopy. As a programmer, I also know how right } he } is in his outrage at such assertions from a manufacturer. } } It's clear from what he is being told that the programmers at DI are } simply } doing a screen dump to TIFF, using the image data written to the screen } object. This is unfortunate as the resolution will also be limited to } that } of the screen. The TIFF file structure was intentionally designed to be } open and simple in order to be a widely used standard. A directory } contains the location of file elements, a number of 'tags' are written } that } describe the file contents and the data is written to the file in a simple } } format. } } Ideally, when writing a TIFF file from a program like this, all acquired } data will be written to the file as a graphical representation that uses } the same resolution and data as that of the original scans. Programs used } } later in the presentation can then adjust the image for whatever needs you } } may have. The TIFF standards allow for easy methods to write this data to } } file in a way that can be understood by any programs that also follow TIFF } } standards. In our work, TIFF is severely limited in several ways, but is } currently the best method to transfer image data. } } Scanning probe methods create data that is not generally depicted as it } is. } The Z axis data, or intensity of a two dimensional image, is normally } translated, as well as the X and Y data, into a rotationally translated } image representing surface topography. Thus the data collected needs this } } imaging translation for presentation. } } Windows gives you various canvasses to draw image data on - the screen and } } printer are two better known examples. When drawing to any of these } canvases, the first job is to determine their capabilities, i.e. } resolution, and adjust your drawing to those limitations. But you can } also } create 'phantom' canvases that have arbitrary resolutions. These are } basically memory spaces that the image data is written to. Once they are } completed, you have a set of data that is appropriate for directly } exporting to TIFF format. This background operation can be completed in a } } fraction of a second and a TIFF file created in a second or two, depending } } on the size. } } I hope this gives enough of a hint to the DI programmers on how to do it, } if not please feel free fire their asses or have them contact me. This is } } an egregious situation for a company who's livelihood relies on computers. } } Just so you know, these are my own opinions and thoughts, and I am my own } employer. I always call it like I see it, and what I see here stinks. } } } Allen R. Sampson } Advanced Research Systems } 317 North 4th. Street } St. Charles, Illinois 60174 } } phone (630) 513-7093 fax (630) 513-7092 http://www.sem.com } } } On Monday, September 23, 2002 12:51 PM, John Mansfield [SMTP:jfmjfm-at-umic } h.edu] wrote: } } ------------------------------------------------------------------------ } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } } -----------------------------------------------------------------------. } } } } } } We have had a Nanoscope AFM since about 1994 and one of the features the } } students use in the software is the simple TIFF export function that } } converts just the image data to a grayscale (or color) TIFF image. } } } } We recently upgraded the software on both of our AFM systems to version } } 5.12r3. The TIFF export menu is still there but it doesn?t let you } export } } just the image data, now you have to export the whole screen and then } use } } another image processing program to extract just the image data! In the } } manual for this version it says that you can do just the image but there } } is } } no option for it in the software. } } } } I called DI and asked about this and the tech support guy didn?t know } why } it } } wasn't there and went to ask the programmers and here is the exact reply } } I } } got: } } } } "As far as the Tiff export goes, I talked to some of our software guys. } They } } tell me the File export for the TIFF never worked very well so they took } } it } } out. But, the file can be cropped in PhotoShop." } } } } Well, we had been using it for nearly 8 years, but I guess we are no } judges } } of how well it works! So they arbitrarily changed the functionality of } the } } software and didn?t even both to change the manual or tell anyone! They } } seem to be able to save the whole screen easily enough, but not the file } } data, how weird is that? } } Even I could program the saving of a simple TIFF file, but apparently } this } } is beyond the software engineers at DI. I wrote back and asked for an } } explanation and was promptly ignored. So I thought this tirade to the } net } } community might wake up someone at DI. } } } } Just so you know, these are my opinions and thoughts, however } unreasoanable, } } my employer has no connection to them whatsoever. } } } } } } -- } } John Mansfield PhD MInstP } } North Campus Electron Microbeam Analysis Laboratory } } 417 SRB, University of Michigan } } 2455 Hayward, Ann Arbor MI 48109-2143 } } Phone: (734) 936-3352 FAX (734) 763-2282 Cell. Phone: (734) 834-3913 } } (Leaving a phone message at 936-3352 is preferable to 834-3913) } } Email: jfmjfm-at-engin.umich.edu } } URL: http://emalwww.engin.umich.edu/people/jfmjfm/jfmjfm.html } } Location: Lat. 42! 16' 48" Long. 83! 43' 48" } } } } } } } } } } } } } } } } } }
I was thinking about printers another day. We do have sort of central facility with super-duper Tektronix dye-sub and color-laser. Dye-sub prints tends to fade (controversy to the previous posting) and our particular printer is slow. Plus $3+ cost for each print... Keeping in mind that most publishers accept now digital format... For myself I decided to use laser-color (somehow it works better than B&W laser) for drafts (quick and very reasonable quality, plus CHEAP) and ink jet for near-photo quality prints. Right now I am setting up Epson 890 photo printer. I am going to use archival quality photo paper (more than 20 years image life) and 'gray-ink' Lyson cartridges. "Gray-ink" supposed to deliver outstanding image quality (if did not kill printer's head) and extended image life. My current situation is that Epson printer I've received a few days ago is defective and will be replaced soon (I hope). I'll report (if anybody interesting) my progress with 'gray-inks'. Sergey
At 12:12 PM 9/24/02, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
_____________________________________
Sergey Ryazantsev Ph. D. Electron Microscopy UCLA School of Medicine Department of Biological Chemistry Box 951737 Los Angeles, CA 90095-1737
Vulgarity is %#&(*$-at-&&$!!!!, and &*(^&*$%(&*($.
And how would vulgarity weaken the force of his argument, anyway?
Let's not be toooooo precious.
cheers
rtch
} From: "David_Bell-at-millipore.com"-at-sparc5.microscopy.com To: "ars-at-sem.com" {ars-at-sem.com} Copies to: jfmjfm-at-umich.edu, microscopy-at-microscopy.com
Dear Jonathon,
Since most of our images are collected digitally, we too have just refurbished our large darkroom into a fluorescence microscopy lab. Yes, lots of our users print out images on their own computers, and we have several inkjets for what I'd call "rough" prints, plus a videoprinter on the SEM, but for "good" printing, we use a central dye-sub printer, and only for those journals that still require prints to copy from or that specify that inkjet prints won't be accepted. So many journals now insist on electronic submission of everything so it seems that producing a stunning print isn't required for this any more. A pity, because some high profile journals are publishing some pretty mediocre quality images, and occasionally publish appalling images - pixellated, odd colours, etc.
my 2c (US1c) worth
} } Hi: } } I missed MSA this year (fell off my bike, broke some things) so I didn't } get a chance to catch up on the latest and greatest regarding the current } state of the art for printing digital images etc. } } Here's my dilema: We have a fancy dye sub printer, but it just broke and } needs repair. We have had it since 1996 and it got lots of use in the first } 4 or 5 years, but business has fallen off lately, like down to one or two } uses in the last several months. I am trying to figure out what is } happening, my guess is that everyone is using some cheap new ink jets in } their own lab to do their printing. We are a small central services type } lab, our users visit us to use the instruments, then take their image files } with them. The dye sub used to get a lot of use from all kinds of people on } campus, but no longer. } } So, what's up with printing? Do I get the dye sub fixed, or do I save the } $$ and buy a couple of photo ink jet things to do its job? There has been a } major transformation in imaging technologies here, our darkroom is } practically abandoned, the dye sub is mostly idle etc. Has printing become } a distributed resource where everyone does it independently, or have some } just given up on printing altogether and everything gets distributed and } submitted in electronic form? } } Just curious. } } Jonathan Krupp } Microscopy & Imaging Lab } University of California } Santa Cruz, CA 95064 } (831) 459-2477 } jmkrupp-at-cats.ucsc.edu
Rosemary White rosemary.white-at-csiro.au Microscopy Centre fax 61- 2 6246 5000 CSIRO Plant Industry ph. 61- 2 6246 5475 or GPO Box 1600 mob. 61- 0402 835 973 Canberra, ACT 2601, Australia
We are in the process of setting up a new lab and "inherited" some printers with some of the equipment. I was also involved in a extensive printer comparison some time ago. My experience is that for normal cheap BW prints the laser 1200 dpi works fine and is fast. On the other hand the Tektronix Phaser does a good job both with colour and BW prints. With the black wax blocs for free it is by far the cheapest prints for BW since it cost only the paper. The images are sensitive to high temperatures e.g.. you can not laminate them! Fading does not appear to be a problem. Personally I am not a inkjet fan. The cartridges are expensive and to get really good images special paper is needed. The dye sub is just to expensive for us here in Botswana.
These are my views only.
Mr S. H. Coetzee Electron Microscope Unit University of Botswana Private Bag 0022 Gaborone Botswana
} -----Original Message----- } From: Stanley L. Flegler [mailto:flegler-at-pilot.msu.edu] } Sent: Tuesday, September 24, 2002 8:04 PM } To: Microscopy-at-sparc5.microscopy.com } Subject: Re: Printers, again } } } -------------------------------------------------------------- } ---------- } The Microscopy ListServer -- Sponsor: The Microscopy Society } of America } To Subscribe/Unsubscribe -- Send Email to } ListServer-at-MSA.Microscopy.Com } On-Line Help } http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -------------------------------------------------------------- } ---------. } } } Jonathan: } } In reference to printers, we are a university core facility } and serve a } broad spectrum of student and faculty users from 45 different } departments. } We have laser jet, ink jet, dye sub, and silver halide } digital printers. } The dye sub has received less and less use as the years have } gone by. It } is a Tektronix Phaser 440 which at one time was the work horse of the } graphic arts industry. However, Tektronix completely dropped } out of the } dye sub market over a year ago. In fact, we can no longer } buy supplies for } it. } } Most students now incorporate images directly into thesis } text and print on } a laser jet or ink jet printer. More and more journals are } accepting and } even preferring electronic submission. However, there are a } substantial } number of users and journals that insist on photographic } quality output. } These users have switched to our silver halide digital printer, a Fuji } Pictrography 3000. The output from this is a photo in the } true sense of } the word because it uses silver halide technology similar to } a photograph. } In my opinion, it is far better than we ever got from the dye } sub printer. } Many professional photo labs are buying these for users that } want the best } possible output. } } This has been our experience. Hope it helps. } } Stanley L. Flegler, Director } Center for Advanced Microscopy } Michigan State University }
using a WDX spectrometer you will have the problem with hudge geometry factors due to focussing principles with Rowland circle. The absolute detector efficiency depends very strong from the surface point, exciting from the electron beam. The differences are higher with lover magnifications, because the covered area is larger. You are able to make X-ray maps with WDX and lower magnification only using stage control scanning! In this case, the absolute efficiency of the WDX spectrometer does not have any changes (everytimes the same geometry for the each point)
Using an EDX spectrometer the efficiency changing is some orders of magnitude lower than with WDX . But with low magnifications low gradients of intensity changings in the maps are visible, too (no changing of element concentration). The effect is higher with very short distances between specimen and detector. There are two ways to avoid the gradient: - retract the X-ray spectrometer to higher specimen - detector distances (of course count rates are going down) - you make a additional map setting one window to element freee bremsstrahlung (background) region. After the mapping you have to process all element maps with special program. You have to divide all images through the bremsstrahlung map. The resulting maps are free from geometrical effects but are a little bit more noisy (depends from measuring time for all maps).
Dear Roy, using a WDX spectrometer you will have the problem with huge geometry factors due to focus principles of Rowland circle. The absolute detector efficiency depends very strong from the surface point, which was excited from the electron beam. The differences are higher with lower magnifications, because the covered area is larger. Only using stage control scanning it is possible to make X-ray maps with WDX with lower magnification! In this case, the absolute efficiency of the WDX spectrometer does not have any changes (every times the same geometry for each point).
Using an EDX spectrometer the efficiency changes are lower than with WDX . But with low magnifications low gradients of intensity in the maps are visible, too (no changing due to element concentration). The effect is higher with very short distances between specimen and detector. There are two ways to avoid the gradient: - Retract the EDX X-ray spectrometer to higher distances between specimen and detector (of course count rates are going down) - You take an additional map of an energy region of bremsstrahlung background (background free of element lines). After the mapping you have to process all element maps with special program. You have to divide (!) all images through the bremsstrahlung image. The resulting maps are free from geometrical effects but are a little bit more noisy (measuring time depending for all maps).
I hope, these hints are useful for you.
Frank Eggert
"Beavers, Roy" wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } Group } } I have been having trouble collecting film based elemental X-ray maps on my Jeol 733 at a magnification of 40X. The map of a mineral grain that fills the screen at this mag (2.5mmx2.5mm?) only shows a concentration of dots diagonally near the center of the grain. I suspect I may be beyond the area in which I can collect X-rays or someting is misaligned. Any comments will be appreciated. } } Thanks } } Roy Beavers } Southern Methodist University } Department of Geological Sciences } P.O. Box 750395 } Dallas, Tx. 75275 } Voice: 214-768-2756 } Fax: 214-768-2701 } Email: rbeavers-at-mail.smu.edu
.. Sorry, my first mail contains the text twice, a funny first version and the final text. Now the final text only: ----------------------------------------------------------------------------------------------------------
Dear Roy, using a WDX spectrometer you will have the problem with huge geometry factors due to focus principles of Rowland circle. The absolute detector efficiency depends very strong from the surface point, which was excited from the electron beam. The differences are higher with lower magnifications, because the covered area is larger. Only using stage control scanning it is possible to make X-ray maps with WDX with lower magnification! In this case, the absolute efficiency of the WDX spectrometer does not have any changes (every times the same geometry for each point).
Using an EDX spectrometer the efficiency changes are lower than with WDX . But with low magnifications low gradients of intensity in the maps are visible, too (no changing due to element concentration). The effect is higher with very short distances between specimen and detector. There are two ways to avoid the gradient: - Retract the EDX X-ray spectrometer to higher distances between specimen and detector (of course count rates are going down) - You take an additional map of an energy region of bremsstrahlung background (background free of element lines). After the mapping you have to process all element maps with special program. You have to divide (!) all images through the bremsstrahlung image. The resulting maps are free from geometrical effects but are a little bit more noisy (measuring time depending for all maps).
I hope, these hints are useful for you.
Frank Eggert
"Beavers, Roy" wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } Group } } I have been having trouble collecting film based elemental X-ray maps on my Jeol 733 at a magnification of 40X. The map of a mineral grain that fills the screen at this mag (2.5mmx2.5mm?) only shows a concentration of dots diagonally near the center of the grain. I suspect I may be beyond the area in which I can collect X-rays or someting is misaligned. Any comments will be appreciated. } } Thanks } } Roy Beavers } Southern Methodist University } Department of Geological Sciences } P.O. Box 750395 } Dallas, Tx. 75275 } Voice: 214-768-2756 } Fax: 214-768-2701 } Email: rbeavers-at-mail.smu.edu
Rosemary has highlighted a point which has been of great concern to me as a manager of an EM lab in the dawning (dawned !) digital era. With the distribution of images electronically, locally or to journals afar, we no longer have the same level of final, critical, control of the quality of the image. I guess that there is no ready solution just the passing of an age - though it is perhaps dubious that we had that much 'control' over the final rendering anyway !!
Tony
Tony Bruton Head, Centre for Electron Microscopy University of Natal, Pietermaritzburg Tel +27 (0) 33 260 5155 Fax +27 (0) 33 260 5776 Mob. 082 782 9640 website: www.nu.ac.za/microscopy.asp Email: bruton-at-nu.ac.za Postal address; Private Bag X01, Scottsville, 3209 KwaZulu-Natal South Africa
} } } Rosemary White {rosemary.white-at-csiro.au} 09/25/02 08:11AM } } } ------------------------------------------------------------------------ The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Dear Jonathon,
Since most of our images are collected digitally, we too have just refurbished our large darkroom into a fluorescence microscopy lab. Yes, lots of our users print out images on their own computers, and we have several inkjets for what I'd call "rough" prints, plus a videoprinter on the SEM, but for "good" printing, we use a central dye-sub printer, and only for those journals that still require prints to copy from or that specify that inkjet prints won't be accepted. So many journals now insist on electronic submission of everything so it seems that producing a stunning print isn't required for this any more. A pity, because some high profile journals are publishing some pretty mediocre quality images, and occasionally publish appalling images - pixellated, odd colours, etc.
my 2c (US1c) worth
} } Hi: } } I missed MSA this year (fell off my bike, broke some things) so I didn't } get a chance to catch up on the latest and greatest regarding the current } state of the art for printing digital images etc. } } Here's my dilema: We have a fancy dye sub printer, but it just broke and } needs repair. We have had it since 1996 and it got lots of use in the first } 4 or 5 years, but business has fallen off lately, like down to one or two } uses in the last several months. I am trying to figure out what is } happening, my guess is that everyone is using some cheap new ink jets in } their own lab to do their printing. We are a small central services type } lab, our users visit us to use the instruments, then take their image files } with them. The dye sub used to get a lot of use from all kinds of people on } campus, but no longer. } } So, what's up with printing? Do I get the dye sub fixed, or do I save the } $$ and buy a couple of photo ink jet things to do its job? There has been a } major transformation in imaging technologies here, our darkroom is } practically abandoned, the dye sub is mostly idle etc. Has printing become } a distributed resource where everyone does it independently, or have some } just given up on printing altogether and everything gets distributed and } submitted in electronic form? } } Just curious. } } Jonathan Krupp } Microscopy & Imaging Lab } University of California } Santa Cruz, CA 95064 } (831) 459-2477 } jmkrupp-at-cats.ucsc.edu
Rosemary White rosemary.white-at-csiro.au Microscopy Centre fax 61- 2 6246 5000 CSIRO Plant Industry ph. 61- 2 6246 5475 or GPO Box 1600 mob. 61- 0402 835 973 Canberra, ACT 2601, Australia
I am currently investigating the properties of a permanent magnetic material. I need to distinguish between Nd-Fe-B particles, epoxy binder and porosities on BSE images obtained on metallographic sections. No problem in singling out the Nd-Fe-B, but do any of you have a suggestion of how to pick up the porosities?
What we have tried up till now is to fill out the sectioned pores with a mix of epoxy and fine silicon powder followed by repolishing to the same level. No succes - the particles were too coarse. I vaguely remember that I have heard about "doped epoxy resins" for this kind of purpose. Perhaps some of you know a recipe or supplier.
Thank you,
Henning Sund Sørensen Materials- and Process Consultant Technology Centre Danfoss A/S 6430 Nordborg, Denmark
We have the PiezographyBW gray scale mods for an Epson 860 printer. This replaces the color inkjet cartridges with gray scale cartridges. As part of the package they provide a PhotoShop plugin to drive the printer (rather than the default Epson "gray" scale driver). On Photo quality paper, the prints are outstanding--fantastic gray scale discrimination, no pixelation! Using a 10X loupe, I can't see any pixelation of the image! The inks are pigments rather than dyes, so they are of archival quality (i.e. won't fade)
It isn't real fast, but for {$400US, we got the printer and the Piezography kit.
Just a satisfied customer...
Henk Colijn
At 07:47 PM 9/24/2002 -0700, Sergey Ryazantsev wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Hendrik O. Colijn colijn.1-at-osu.edu Campus Electron Optics Facility Ohio State University (614) 292-0674 http://www.ceof.ohio-state.edu Fools are pleased when they discover error. The wise are pleased when they discover truth.
In the early 1980s, I was looking for a doped epoxy to provide contrast in backscattered imaging between epoxy and coal. There was often a very slight contrast, but we needed something more marked to facilitate image analysis.
I came across papers that suggested dissolving bromoform or iodaform in epoxy resin to raise the atomic number. We chose iodaform. I think the recipe was about 15% iodaform by weight in epoxy resin. (I think 18% produced a saturated solution. Certainly less than 15% could be used.) We warmed the mixture to aid dissolution. I could then store and use the resin more or less as normal. I may have had to adjust (decrease) the amount of hardener, but I think we may have also changed epoxy formulations about the same time from a 4:1 mix to an 8:1 mix. Otherwise, the material behaved the same.
Be advised that iodaform comes with plenty of health warnings. Be sure to read and heed the advisories.
Warren Straszheim
with At 02:33 PM 9/25/02 +0200, you wrote:
} Dear Listers, } } I am currently investigating the properties of a permanent magnetic } material. } I need to distinguish between Nd-Fe-B particles, epoxy binder and porosities } on BSE images obtained on metallographic sections. No problem in singling } out the Nd-Fe-B, but do any of you have a suggestion of how to pick up the } porosities? } } What we have tried up till now is to fill out the sectioned pores with a mix } of epoxy and fine silicon powder followed by repolishing to the same level. } No succes - the particles were too coarse. } I vaguely remember that I have heard about "doped epoxy resins" for this } kind of purpose. Perhaps some of you know a recipe or supplier. } } Thank you, } } Henning Sund Sørensen } Materials- and Process Consultant } Technology Centre } Danfoss A/S } 6430 Nordborg, Denmark
List, From the single user's perspective, I'd like to put in a plug for inkjets. I have an Epson 970. I am AMAZED at how well this thing prints. I keep three grades of paper on hand, two are fancier types of basic zerox paper, and the third is photopaper. The printer has controls to adjust the quality and match to the paper. The fancier white papers are not expensive (at least in USA) and the output on them is wonderful and perfect for reviewer figures, grant proposals (14 copies!), and handles color or black and white with no trouble. And when I put in photopaper the output is phenomenal. I have never even for a microsec considered using the fancy printers in our core facility. For my own needs, the cartridges last long enough.
No financial ties to any printer co (or to anything else for that matter, 8-).
1. Do you have the energy of interest properly selected for mapping? That is, selecting the energy at which the analyzer will place a dot on the map. This is a software selection.
2. Are your counts/sec. high enough?
3. Is your beam energy high enough for excitation of the spectral line you are trying to map?
4. Is the EDX detector's "field of view" catching the x-ray photons. This will be some solid angle which is a function of the detector area, probe angle etc.
And just a suggestion but put the SEM in a "spot mode" and see if you detect the element of interest above the background noise. Are you mapping multiple elements simultaneously or just one? What do you expect the elemental concentration to be? Finally, what is the element and in what elemental matrix is it in?
Peter
-----Original Message----- } From: Beavers, Roy [mailto:rbeavers-at-post.cis.smu.edu] Sent: Tuesday, September 24, 2002 11:50 AM To: Microscopy Listserver; Microprobe List (E-mail)
Group
I have been having trouble collecting film based elemental X-ray maps on my Jeol 733 at a magnification of 40X. The map of a mineral grain that fills the screen at this mag (2.5mmx2.5mm?) only shows a concentration of dots diagonally near the center of the grain. I suspect I may be beyond the area in which I can collect X-rays or someting is misaligned. Any comments will be appreciated.
Thanks
Roy Beavers Southern Methodist University Department of Geological Sciences P.O. Box 750395 Dallas, Tx. 75275 Voice: 214-768-2756 Fax: 214-768-2701 Email: rbeavers-at-mail.smu.edu
I'm curious about any experiences people may have had with using glycol methacrylate, or similar resins, for TEM of biological tissue. Specifically, we are concerned with retinal tissue. We have found that we have seen flatter and more consistently stained thick sections from GMA embedded retina from another lab. We'd like to know if the quality of the EM work done with resin is good enough to warrant switching over from our standard EPON, EPON/Spurr's, or EPON/Araldite protocols, in order to get better quality LM of thicks.
My own opinion is that if TEM is part of the procedure, we should optimize the TEM protocols, even if the thicks don't look quite as nice. Running two protocols, one for LM and one for TEM, is not an option for us in this case.
We will run some tests, but any opinions or experiences are very welcome.
Thanks a bunch.
Randy
Randy Tindall EM Specialist Electron Microscopy Core Facility W122 Veterinary Medicine University of Missouri Columbia, MO 65211 Tel: (573) 882-8304 Fax: (573) 884-5414 Email: tindallr-at-missouri.edu Web: http://www.biotech.missouri.edu/emc/
Dear Colleagues, We would like to make some experiments on analysis of old paper samples serving as a support for oil painting. I would be grateful for any information concerning the sample preparation for SEM (we have low vacuum Jeol 5500 LV)
Thank you
Jan
dr. Jan Rutkowski Academy of Fine Arts Conservation Dept, Physics Lab ul. Smolensk 9 31-108 Krakow, Poland
Henning Polysciences sell lead, barium and zinc acrylates which can be used to make radio-opaque acrylic polymers. Many other metal-methacrylates / acrylates are known, probably commercially available, including Li, Na, K, Ca, Y, Zr, Ag, Cu, Fe, Cr, etc Europium methacrylate is apparently fluorescent.
These may provide a bse or xray signal. I have considered using them, but the polymerization techniques for barium and lead methacrylates sound too hairy, probably involving ionising radiation capable of penetrating your metals.
Are your voids big enough to image using fluorescence microscopy? If so, doping the epoxy with a fluorescent dye may work. see e.g.
or Fischer, U., B. Kulli, H. Flühler and P. Marschall (1996). Determining the pore structure of shear zone granite samples by means imbibition with fluorescent resin and image analysis procedures, Nagra, Wettingen, Interner Bericht 96-79, 39 Seiten.
Chris
} From: Sørensen Henning Sund {Henning.S-at-danfoss.com} To: Microscopy-at-sparc5.microscopy.com
Henning, I assume that you want to be able to distinguish between particles, the space between particles, and the pores that are in the particles.
I have found, as you, that powders mixed with epoxy do not work.
Struers sells a fluorescent dye that you can add to epoxy. I have also used a blue dye (Oil blue) that is used in the petroleum industry to color lubricants and fuels. This is very soluble in epoxy.
Everett Ramer Cellomics, Inc. Pittsburgh, PA
-----Original Message----- } From: Sørensen Henning Sund [mailto:Henning.S-at-danfoss.com] Sent: Wednesday, September 25, 2002 8:34 AM To: Microscopy-at-sparc5.microscopy.com
Dear Listers,
I am currently investigating the properties of a permanent magnetic material. I need to distinguish between Nd-Fe-B particles, epoxy binder and porosities on BSE images obtained on metallographic sections. No problem in singling out the Nd-Fe-B, but do any of you have a suggestion of how to pick up the porosities?
What we have tried up till now is to fill out the sectioned pores with a mix of epoxy and fine silicon powder followed by repolishing to the same level. No succes - the particles were too coarse. I vaguely remember that I have heard about "doped epoxy resins" for this kind of purpose. Perhaps some of you know a recipe or supplier.
Thank you,
Henning Sund Sørensen Materials- and Process Consultant Technology Centre Danfoss A/S 6430 Nordborg, Denmark
Henning, Sorry, I thought you were using optical microscopy.
For SEM work you can add iodoform (CHI3) to epoxy to increase the contrast between the epoxy you use for mounting and the epoxy you use to fill the pores.
Everett Ramer
------------------------------------------------------------------------ The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Dear Listers,
I am currently investigating the properties of a permanent magnetic material. I need to distinguish between Nd-Fe-B particles, epoxy binder and porosities on BSE images obtained on metallographic sections. No problem in singling out the Nd-Fe-B, but do any of you have a suggestion of how to pick up the porosities?
What we have tried up till now is to fill out the sectioned pores with a mix of epoxy and fine silicon powder followed by repolishing to the same level. No succes - the particles were too coarse. I vaguely remember that I have heard about "doped epoxy resins" for this kind of purpose. Perhaps some of you know a recipe or supplier.
Thank you,
Henning Sund Sørensen Materials- and Process Consultant Technology Centre Danfoss A/S 6430 Nordborg, Denmark
Quite so! Tony has hit the nail on the head here. Over the years I've seen "real" photographic plates that I was extremely proud of look really rather awful in publication, and those that I wrote off as "the best that could be done with what I had" turn out not so bad looking in the end. The same goes for digital plates. In fact, some of the better ones turned out to have been scanned from inkjet prints submitted for review! I think the skill of the guys in the print shop have a lot to do with the final output.
My 3.3 cents (Canadian)....
Jim
--
James M. Ehrman Digital Microscopy Facility Mount Allison University Sackville, NB E4L 1G7 CANADA
Rosemary has highlighted a point which has been of great concern to me as a manager of an EM lab in the dawning (dawned !) digital era. With the distribution of images electronically, locally or to journals afar, we no longer have the same level of final, critical, control of the quality of the image. I guess that there is no ready solution just the passing of an age - though it is perhaps dubious that we had that much 'control' over the final rendering anyway !!
Tony
Tony Bruton Head, Centre for Electron Microscopy University of Natal, Pietermaritzburg Tel +27 (0) 33 260 5155 Fax +27 (0) 33 260 5776 Mob. 082 782 9640 website: www.nu.ac.za/microscopy.asp Email: bruton-at-nu.ac.za Postal address; Private Bag X01, Scottsville, 3209 KwaZulu-Natal South Africa
Our facility employs several different printer technologies to display our work. Ultimately the final use of the printed material will determine which print technology is select. For example, routine images / spectra are printed on HP laser printers (B & W) or deskjet printers (color). When higher quality is necessary we use a Kodak 8650 with "extra-life" ribbons (Black-BX or Color-CMYX). For high volume B & W print jobs that require a higher quality than our laserjet technologies we use a codonics NP1650 (thermal-directvista paper) printer. And finally, we occasionally use a color laser to output color prints or reports containing color information. The vast majority of our work is run through the laser and inkject printers, however, our work is enhanced by having availability of all the technologies. The single most import upgrade to our laboratory (in regard to printing) has been the ability to access printers from throughout the R & D building. We have access to dozens of laser and inkjet printers, including color laser printers. We are fortunate to have a 1996 vintage Kodak that has performed flawlessly and a codonics that was purchased 2 years ago which also has performed satisfactorily. Bottom line, if you have them, use them!
PS Sergey, it has been my experience that Kodak's extra-life coating assists in protecting the image from minor water damage, bleeding, and fading commonly encountered with the 3 color CMY or 4 color CMYK ribbons. This is available in either black or CMY versions only, to my knowledge there is no CMYK version with the extra-life option. Expensive.....definitely! But in our line of work the quality of the work is often judged by the presentation of the results, as much, or more so than the content of the data. Sad but true.
} John A. Robson } _____________________________________________________ } } Boehringer Ingelheim Pharmaceuticals, Inc. } Research and Development } 900 Ridgebury Road / P. O. Box 368 } Ridgefield, CT 06877-0368 } } phone: 203.798.5640 } fax: 203.798.5698 } email: jrobson-at-rdg.boehringer-ingelheim.com } } } } -----Original Message----- } From: Sergey Ryazantsev [SMTP:sryazant-at-ucla.edu] } Sent: Tuesday, September 24, 2002 10:48 PM } To: Microscopy-at-sparc5.microscopy.com } Subject: Re: Printers, again } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } I was thinking about printers another day. We do have sort of central } facility with super-duper Tektronix dye-sub and } color-laser. Dye-sub prints tends to fade (controversy to the previous } posting) and our particular printer is slow. Plus $3+ cost for each } print... Keeping in mind that most publishers accept now digital } format... } For myself I decided to use laser-color (somehow it works better than B&W } laser) for drafts (quick and very reasonable quality, plus CHEAP) and ink } jet for near-photo quality prints. Right now I am setting up Epson 890 } photo printer. I am going to use archival quality photo paper (more than } 20 years image life) and 'gray-ink' Lyson cartridges. "Gray-ink" supposed } } to deliver outstanding image quality (if did not kill printer's head) and } extended image life. My current situation is that Epson printer I've } received a few days ago is defective and will be replaced soon (I } hope). I'll report (if anybody interesting) my progress with } 'gray-inks'. Sergey } } At 12:12 PM 9/24/02, you wrote: } } ------------------------------------------------------------------------ } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } } -----------------------------------------------------------------------. } } } } } } Measure the time it takes to print an image of a Codonics 1600 (if you } can } } get it to work) and then measure the time it takes to print an image on } an } } Epson 980 or similar (the one's we happen to use) and then look at the } cost } } difference and see that I'd go for the Epson anytime. They're } disposable. } } } } Again, MY opinion, no one else's! } } } } On 9/24/02 2:23 PM, "Warren E Straszheim" {wesaia-at-iastate.edu} wrote: } } } } } } ------------------------------------------------------------------------ } } } The Microscopy ListServer -- Sponsor: The Microscopy Society of } America } } } To Subscribe/Unsubscribe -- Send Email to } ListServer-at-MSA.Microscopy.Com } } } On-Line Help } http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } } } } -----------------------------------------------------------------------. } } } } } } } } } I think I would concur with your guesses. Everyone is probably doing } it on } } } their own. } } } } } } Current inkjet printers CAN do a quite good job rendering images on } good } } } paper. I have heard John Mc Kenzie recommend them at his seminars. } Granted } } } that many inkjets are still slow compared to other technologies. John } even } } } suggests setting up a bank of relatively cheap inkjets to share the } jobs } } } and keep through-put up. We haven't gone that route yet. } } } } } } Users may also be settling for mediocre prints from their own printers } not } } } knowing what quality is available. We have an aging Lexmark Optra Rt+ } that } } } does a quite good job of printing B/W images on bright white paper. I } just } } } passed some prints from it on to a user who had tried printing images } on } } } his own printer. He much preferred our quality once he saw the prints. } He } } } just assumed, falsely in this case, that he could get the same quality } on } } } his own. Maybe you should post a classic image next to your printer so } your } } } users see what you can do. } } } } } } But having said that, I probably would consider retiring the printer } } } depending on the cost of repair. Printer technology has come a long } way in } } } recent years and the new stuff generally does better for cheaper. } } } } } } Warren } } } } } } At 10:03 AM 9/24/02 -0700, you wrote: } } } } } } } Hi: } } } } } } } } I missed MSA this year (fell off my bike, broke some things) so I } didn't } } } } get a chance to catch up on the latest and greatest regarding the } current } } } } state of the art for printing digital images etc. } } } } } } } } Here's my dilema: We have a fancy dye sub printer, but it just broke } and } } } } needs repair. We have had it since 1996 and it got lots of use in the } } } first } } } } 4 or 5 years, but business has fallen off lately, like down to one or } two } } } } uses in the last several months. I am trying to figure out what is } } } } happening, my guess is that everyone is using some cheap new ink jets } in } } } } their own lab to do their printing. We are a small central services } type } } } } lab, our users visit us to use the instruments, then take their image } } } files } } } } with them. The dye sub used to get a lot of use from all kinds of } } people on } } } } campus, but no longer. } } } } } } } } So, what's up with printing? Do I get the dye sub fixed, or do I save } the } } } } $$ and buy a couple of photo ink jet things to do its job? There has } } been a } } } } major transformation in imaging technologies here, our darkroom is } } } } practically abandoned, the dye sub is mostly idle etc. Has printing } become } } } } a distributed resource where everyone does it independently, or have } some } } } } just given up on printing altogether and everything gets distributed } and } } } } submitted in electronic form? } } } } } } } } Just curious. } } } } } } } } Jonathan Krupp } } } } Microscopy & Imaging Lab } } } } University of California } } } } Santa Cruz, CA 95064 } } } } (831) 459-2477 } } } } jmkrupp-at-cats.ucsc.edu } } } } } } ------------------------------------------- } } } No files should be attached to this message } } } ------------------------------------------- } } } Warren E. Straszheim, Ph.D. } } } Materials Analysis and Research Lab } } } Iowa State University } } } 23 Town Engineering } } } Ames IA, 50011-3232 } } } } } } Ph: 515-294-8187 } } } FAX: 515-294-4563 } } } } } } E-Mail: wesaia-at-iastate.edu } } } Web: www.marl.iastate.edu } } } } } } Scanning electron microscopy, x-ray analysis, and image analysis of } } materials } } } Computer applications and networking } } } } } } } } } } } } } } } } -- } } John Mansfield PhD MInstP } } North Campus Electron Microbeam Analysis Laboratory } } 417 SRB, University of Michigan } } 2455 Hayward, Ann Arbor MI 48109-2143 } } Phone: (734) 936-3352 FAX (734) 763-2282 Cell. Phone: (734) 834-3913 } } (Leaving a phone message at 936-3352 is preferable to 834-3913) } } Email: jfmjfm-at-engin.umich.edu } } URL: http://emalwww.engin.umich.edu/people/jfmjfm/jfmjfm.html } } Location: Lat. 42! 16' 48" Long. 83! 43' 48" } } _____________________________________ } } Sergey Ryazantsev Ph. D. } Electron Microscopy } UCLA School of Medicine } Department of Biological Chemistry } Box 951737 } Los Angeles, CA 90095-1737 } } Phone: (310) 825-1144 } FAX (departmental): (310) 206-5272 } mailto:sryazant-at-ucla.edu } } } }
To: "Jan Rutkowski" {zerutkow-at-cyf-kr.edu.pl} cc:
years ago, my boss would submit papers to a select handful of journals...those that consistently did an good job of rendering electron micrographs. In those days there were still journals that published pictures in what could be equated with newspaper style, lots of dots. The larger the dots, the poorer the picture. On second thought, maybe things haven't changes all that much! Lee -- Leona Cohen-Gould, M.S. Sr. Staff Associate Director, Electron Microscopy Core Facility Manager, Optical Microscopy Core Facility Joan & Sanford I. Weill Medical College of Cornell University voice (212)746-6146 fax (212)746-8175
We are looking to acquire some additional double replica booklets for use on a Balzers 400T freeze-fracture plant. Would welcome information from vendors or individuals with booklets to dispose of. Johnny Carson Cell Biology/Ultrastructure Facility Center for Environmental Medicine, Asthma, and Lung Biology The University of North Carolina at Chapel Hill e-mail: jcarson-at-med.unc.edu
I like to make presentations with overheads (transparencies, or films). I have had problems with the quality of inkjet printers printing to transparencies. I have tried Epson printers, and they have given the worst results. And, I have tried more than one model. HP inkjet printers are pretty good. A good sublimation dye printer has given me the best results.
-Scott
Scott D. Walck, Ph.D. PPG Industries, Inc. Glass Technology Center P. O. Box 11472 (letters) Guys Run Rd. (packages) Pittsburgh, PA 15238-0472
Walck-at-PPG.com
(412) 820-8651 (office) (412) 820-8515 (fax)
"The opinions expressed are those of Scott D. Walck and not of PPG Industries, Inc. nor of any PPG-associated companies."
-----Original Message----- } From: Tobias Baskin [mailto:BaskinT-at-missouri.edu] Sent: Wednesday, September 25, 2002 10:02 AM To: Microscopy-at-sparc5.microscopy.com
List, From the single user's perspective, I'd like to put in a plug for inkjets. I have an Epson 970. I am AMAZED at how well this thing prints. I keep three grades of paper on hand, two are fancier types of basic zerox paper, and the third is photopaper. The printer has controls to adjust the quality and match to the paper. The fancier white papers are not expensive (at least in USA) and the output on them is wonderful and perfect for reviewer figures, grant proposals (14 copies!), and handles color or black and white with no trouble. And when I put in photopaper the output is phenomenal. I have never even for a microsec considered using the fancy printers in our core facility. For my own needs, the cartridges last long enough.
No financial ties to any printer co (or to anything else for that matter, 8-).
Dear Dr. Sorensen, I have used epoxy doped with Br to track the movement of epoxy while curing composites and bromine staining of lignin to track the pulping of wood. This tracking was done by WDS or EDS, not BSE. In brominating the lignin, the material was just contacted with a bromine solution. The brominated resin was available commercially. It might be easier, in your case, to adjust the brightness and contrast of the BSE detector to show a dark gray for the epoxy binder and black for the porosity. By SE, the pores will show bright rims and the epoxy should not. At 02:33 PM 09/25/2002 +0200, you wrote: } } Dear Listers, } } I am currently investigating the properties of a permanent magnetic } material. } I need to distinguish between Nd-Fe-B particles, epoxy binder and porosities } on BSE images obtained on metallographic sections. No problem in singling } out the Nd-Fe-B, but do any of you have a suggestion of how to pick up the } porosities? } } What we have tried up till now is to fill out the sectioned pores with a mix } of epoxy and fine silicon powder followed by repolishing to the same level. } No succes - the particles were too coarse. } I vaguely remember that I have heard about "doped epoxy resins" for this } kind of purpose. Perhaps some of you know a recipe or supplier. } } Thank you, } } Henning Sund Sørensen } Materials- and Process Consultant } Technology Centre } Danfoss A/S } 6430 Nordborg, Denmark } Regards, Mary
Mary Mager Electron Microscopist Metals and Materials Engineering University of British Columbia 6350 Stores Road Vancouver, B.C. V6T 1Z4 CANADA tel: 604-822-5648 e-mail: mager-at-interchg.ubc.ca
Listers, Thank you for all the help in staining the HIPS with rubber particles. We have been experimenting and found that, with these samples, immersion in 2% OsO4 gave some contrast to the particles. However, the resulting image was not very crisp due to the particles having little edge contrast.
Then we took these same immersion stained samples, sectioned, and vapor stained the sections. This resulted in additional contrast, primarily helping to outline the edges of the rubber phase, which resulted in very nice images.
Vapor staining without prior immersion also worked quite well although the particle staining was not quite as dense. However, we did note more "pulling" of particles throughout the sample. Apparently the immersion in osmium just firmed up the sample enough to section with less distortion just as some of you predicted.
Thanks again for all the advice. Debby
Debby Sherman, Manager Phone: 765-494-6666 Life Science Microscopy Facility FAX: 765-494-5896 Purdue University E-mail: dsherman-at-purdue.edu S-052 Whistler Building West Lafayette, IN 47907
I agree with your sentiment, Ritchie, but you are wrong about what "vulgarity" is. What you have expressed is mere symbolism with no substance. If Allen had been vulgar in any way, we would have heard from the net gods immediately. Since that has not occurred, I must disagree emphatically with the notion that any vulgarity has been used at all. Further, I was dead on with Allen with everything he said until he suggested firing a donkey. I saw no relevance in that part of his argument at all, but then there is nothing in my past that would permit me to claim any programming power, so I may have read that variable name out of context. Finally, my son IS a programmer, and I take issue with the notion that such wonderful folk are ever vulgar, even though they all seem to take great delight in using the phrase "data is" which is, after all, syntactically incorrect.
So, TIFF-UNIX or TIF-WIN to you all, and to all a good night.
Of all the anatomists I know I am among the luckiest. I watched a Technai being assembled all day and will watch a Quanta arrive tomorrow, and I am the only one in line for one, and the operator for both. Since the last SEM I ran was over ten and the TEM over 25, I am a lucky S.O.B.
When Mama spoke about the relationship of cleanliness to Godliness, she was referring to soap, as I recall!
And Allen, I appreciated the lesson in TIFFology despite the zoological miscue.
Fred Monson
Frederick C. Monson, PhD Center for Advanced Scientific Imaging Geology-Astronomy West Chester University of Pennsylvania Schmucker Science Center II South Church street & Rosedale Avenue West Chester, PA, 19383, USA Phone: 610-738-0437 FAX: 610-738-0437 eMail: fmonson-at-wcupa.edu http://darwin.wcupa.edu/casi/ http://www.wcupa.edu/_visitors/
-----Original Message----- } From: Ritchie Sims [mailto:r.sims-at-auckland.ac.nz] Sent: Tuesday, September 24, 2002 11:07 PM To: "David_Bell-at-millipore.com"-at-sparc5.microscopy.com Cc: microscopy-at-microscopy.com
Oh, come on!
That's not vulgarity!
Vulgarity is %#&(*$-at-&&$!!!!, and &*(^&*$%(&*($.
And how would vulgarity weaken the force of his argument, anyway?
Let's not be toooooo precious.
cheers
rtch
} From: "David_Bell-at-millipore.com"-at-sparc5.microscopy.com To: "ars-at-sem.com" {ars-at-sem.com} Copies to: jfmjfm-at-umich.edu, microscopy-at-microscopy.com
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Announcement for 6th Multinational Congress on Microscopy (organised by Croatian, Austrian, Czechslovak, Hungarian, Italian and Slovenian Society for Electron Microscopy) June 1-5, 2003 Pula, Croatia
The Congress is open for the contributions dealing with all aspecs of microscopy topics in materials science, biomedical research and instrumentation.
Please visit the web site
http://www.6mcm.kbsm.hr/
Prof. Andjelka Tonejc Department of Physics Zagreb, Croatia
To all interested in paper: I should have included some references that have been useful to me in my studies of papers. 1.) "New electron and light optical techniques for examining paper making , Donald L. Gibbon, George C. Simon, and Richard C. Cornelius, from TAPPI Journal 10/89. ( discusses the embedding and metallurgical polishing procedures, I don't do the infiltration steps since the vacuum impregnation works better for me )
2.) "Determining paper-coating thickness with electron microscopy and image analysis" , Richard A. Peterson and Christopher L. Williams. from TAPPI Journal 10/92 , ( Discusses using the ultramicrotome for cross-sections)
3.) "The Application of Microtomy in the Paper Industry" , Eckehard Saverin, Claudia Bachie-Stolz, from Jung Application Brief, Leica. ( this has some nice light micrographs of stained paper cross-sections and tips for embedding ) Terry Ellis Hallmark Cards Inc. Kansas City, MO , USA 816-545-6573
we have a Photometrics Sensys CCD camera mounted on our microscope being run via a Power Mac 9600 with a PCI Snapper card. This works good. However, when we have tried to upgrade to a Power Mac G4 (with a new model II PCI card), our system no longer recognizes the camera being there. We supposedly have the correct drivers installed. Has anyone encountered this problem and found a fix?
Robert Underwood U of Washington Dept of Med, Div of Derm Seattle WA
With apologies for tooting my own horn, you might look at....
Rothbard, D.R. (2002) Applied Microscopy for the Paper Industry. Microscopy & Microanalysis 2002, Proceedings, Cambridge University Press, New York, p. 178-179
Rothbard, D.R. (In Press) Electron Microscopy for the Pulp and Paper Industry. In Z. Li (Ed.), Industrial Applications of Electron Microscopy, Marcel Dekker, New York
Also:
OW Gregersen, PO Johnsen, T Helle. Small-scale topographic variations of newsprint surfaces and their effects on printing ink transfer distribution. J. Pulp Paper Sci. 21(10): J331-J336, 1995
A Donald, L Jenkins. Use of environmental scanning electron microscope for observation of the swelling behavior of cellulosic fibers. Scanning 19(2): 92-97, 1997
GJ Williams, JG Drummond. Preparation of large sections for the microscopical study of paper structure. J. Pulp Paper Sci. 26(5): 188-193, 2000
RA Parham. Electron Microscopy of Pulp and Paper. Wood Science. 6(3): 245-255, 1974
David Rothbard Earthborn Solutions rothbardD-at-netscape.net
We have a TMC MICRO-g Anti-Vibration Isolation Platform Model # 65-17171-01 that we used to support a JEOL 100C TEM that we wish to sell. The platform is 86" wide by 71" deep with a seating cut out that is -at- 30" wide narrowing down to 12" and is about 38" deep. System has 4 isolation gimble feet to float the platform. With the feet, it requires an area that is 97" x 82". The weight of unit is about 2200 lbs. Asking $3,000.00 or best offer plus shipping and handling charges. Interested parties should contact
Joe Goodhouse Confocal / EM Core Laboratory Department of Molecular Biology Princeton University 609-258-5432 or
Bill Huston bhuston-at-molbio.princeton.edu 609-258-6205
The three-day intensive hands-on workshop on Image Processing and Measurement presented by John Russ (author of "The Image Processing Handbook" and "Practical Stereology") through the North Carolina State University Department of Continuing and Professional Education is now in its 21st year. The upcoming course dates are November 6-8, 2002, and May 21-23, 2003, in Raleigh, and June 9-11, 2003, at the Danish Technological Institute in Taastrup, Denmark (near Copenhagen). This course has generated highly favorable reviews from the thousands of previous students. The primary focus is on images from various types of microscopy, with practical guidance in correcting imaging defects, enhancing the images for presentation and measurement, and performing stereological meaningful measurements on them. Textbooks and computer software are provided to attendees. Lab sessions with an opportunity to bring your own images makes this course immediately useful and highly productive.
There are still a few openings available for the November session. For full information on the course, including outlines, faculty information, a downloadable brochure, and on-line registration, go to
{http://members.aol.com/ipcourse}
Class size is limited to maintain a high ratio of instructors to students, so make your reservation now. You may also contact Cindy Allen at NCSU Continuing Education, at 919-515-8171
Are there any folks out there that are working with analysis of failure mechanisms or failure potential areas of damascene ICs?
I would appreciate conversing with anyone doing this using FIB and/or SEM. Methods of analyzing damascene structures is at issue. A particular goal is to determine how commercial damascene devices survive in a hostile environment. I know that there are incipient failure mechanisms in small feature size ICs. The issue is to discover and quantify these sufficiently to make them validated.
Off-line responses are invited.
Gary Gaugler, Ph.D. Microtechnics, Inc. Granite Bay, CA
Trouble is Terry they're all just "paper studies" :-)
} } To all interested in paper: } I should have included some references that have been useful to me in } my studies of papers. } 1.) "New electron and light optical techniques for examining paper making , } Donald L. Gibbon, George C. Simon, and Richard C. Cornelius, from TAPPI } Journal 10/89. ( discusses the embedding and metallurgical polishing } procedures, I don't do the infiltration steps since the vacuum impregnation } works better for me ) } } 2.) "Determining paper-coating thickness with electron microscopy and image } analysis" , Richard A. Peterson and Christopher L. Williams. from TAPPI } Journal 10/92 , ( Discusses using the ultramicrotome for cross-sections) } } 3.) "The Application of Microtomy in the Paper Industry" , Eckehard } Saverin, Claudia Bachie-Stolz, from Jung Application Brief, Leica. ( this } has some nice light micrographs of stained paper cross-sections and tips } for embedding ) } Terry Ellis } Hallmark Cards Inc. } Kansas City, MO , USA } 816-545-6573
Roy, The expanations you've gotten concerning the Rowland Circle are correct, hence, if you have an EDS that will detect and map what you're looking for, use it.
40x is getting pretty low in mag, but the following technique has been used to do low mag WDS mapping. Use your electronic raster rotation to make the band of dots horizontal. (If you don't have the raster rotation module, you're out of luck.) Set your scan generator for a single line and move that line to the top of your CRT. Peak the countrate on your spectrometer by changing the spectrometer crystal/detector position and note the position where it peaks. Move the line to the bottom of your CRT and repeak your counts. Note the spectrometer position.
Now you need to do a little calculating. Determine how long your record sweep takes and find a speed for your spectrometer that will take you between the 2 positions determined above. Set the spectrometer for the first position and start it scanning towards the second position at the same time you start the record scan. This won't give a perfect map at very low mags, but it is much better than that little diagonal band.
What you're doing here is playing with the effective position of the Rowland Circle. At low enough mags the system becomes so detuned that you will get a major signal roll-off at both the top and botton of the sweep, but if you need to isolate a particular line or a light element and do it at low mag, or you just don't have an EDS system, this is about the best you can do.
Good luck,
Ken Converse owner Quality Images third party SEM service Delta, PA
Beavers, Roy wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
I have some questions concerning quantitative composition analysis by EDS in a TEM. 1. how do I do the quantitative analysis correctly? Is it a truly standardless method? What precautions should be taken?
2. I checked a EuS sample. I used Eu L lines and S K line. It gives about 70%Eu and 30%S, which is way off the stoicheometric value. The sample is believed to be not far from 50%Eu and 50%S. The result of a GaAs sample seems reasonable. So what is the reason for this result? because of using L lines?
I would appreciate very much help and suggestions on this.
Regards Yan Xin ======================================= Yan Xin (Ph.D) Magnet Science & Technology National High Magnetic Field Laboratory Florida State University 1800 E. Paul Dirac Drive Tallahassee, FL 32310 Tel: (850) 644 1529 Fax: (850) 644 0867 ========================================
Looking for a schematic for a CARY 401 Vibrating Reed Electrometer. If anyone can help please contact me directly. Thanks Roy Beavers Southern Methodist University Department of Geological Sciences P.O. Box 750395 Dallas, Tx. 75275 Voice: 214-768-2756 Fax: 214-768-2701 Email: rbeavers-at-mail.smu.edu
I notice in some catalogs, that one has the option of ordering either Platinum or Molybdenum apertures. what are the advantages and disadvantages between the two?
Stu Smalinskas Senior Metallurgist SKF NATC Plymouth, Michigan
__________________________________________________ Do you Yahoo!? New DSL Internet Access from SBC & Yahoo! http://sbc.yahoo.com
At 10:01 AM 9/27/02 -0500, you wrote: } You didn't say if you were reporting your results as mass fraction or } atomic fraction. The two values will be similar for GaAs since they have } atomic masses of 70 and 75. But Eu has a mass of 152 while S has a mass of } 32, so the results should be about 83:17 by mass. BTW, how do you know the } EuS sample is really a 1:1 stoichiometry?
Warren,
Thanks for the suggestions. They are atomic fractions.
I used the target materials. It was made stoichiometric.
Has anyone tried HP LaserJet 4600 Color Laser Printer for SEM pictures? Its supposed to print 17ppm BW and color with 600dpi with HP Imageret 2400 dpi. Any suggestions, concerns, or recommendations before we decide to purchase one?
You questions (especially number 1) can't be answered properly in an e-mail like this. Very brief and incomplete answers are:
There are lots of things that must be done before you can trust an EDX analysis in the TEM. You need to understand the electron probe characteristics (assuming you are needing high spatial resolution analysis), and any spurious responses from your microscope/X-ray analyzer configuration, as well as any peculiarities in your particular x-ray detector. I don't think these issues are relevant to your particular analysis, though.
The age and manufacturer of your system will determine how trustworthy your "standardless" analyses are - some newer systems give very good results (in some analyses, at least), while others, using older techniques/constants/whatever can be quite questionable. A general "rule of thumb" is that comparing two elements close to each other in the periodic table (such as Ga and As) is more reliable than comparing elements far removed from each other, especially if you are using x-ray lines of different families (as in your case). The only way to be sure is to analyze a sample of known composition (in effect, determine your own standards)
Sample thickness is very important. In your case, the S-K line is at about 2.3 KeV, while the Eu-M absorption edge is at about 1.16KeV. The Eu-L line you are measuring is at 5.85Kev, and the S-K absorption edge is at 2.5KeV. Calculating (from Kurt Heinrich's tables) the mass absorption coefficients for S and Eu in the sample gives 2149 cm^2/gm for S and 244 for Eu. If you are working in a 200KV or 300KV TEM, it would be easy to be in an area thick enough that an absorption correction would be essential. If your sample is bent so that the area you are analyzing is tilted away from the x-ray detector, it will make this problem worse. This effect would tend to give a low S analysis.
Sometimes the microscope geometry can be incorrect (if the sample height is wildly wrong, for example), and this, too, can reduce the intensity of the low-energy lines more than the high energy ones.
These problems of absorption, whether due to thickness or geometry, are easily seen in the shape of the bremsstrahlung background. If there is anyone in your lab who has lots of experience with your particular system, they should be able to look at the spectra and tell at once if the shape of the bremsstrahlung is near-enough correct.
Of course your software must be set up with the correct operating voltage, but that would make only a relatively small change in the result, (as opposed to the situation in the SEM, where the correct voltage is critical).
I don't know about europium compounds, but iron sulphides are not stable under the electron beam. They lose S as time passes. Taking a number of analyses for short times at the same point can demonstrate this (the S content will progressively fall).
I hope I don't depress you too much!!!
Tony.
At 09:56 AM 9/27/2002 -0400, Yan Xin wrote: } I have some questions concerning quantitative composition analysis by EDS } in a TEM. } 1. how do I do the quantitative analysis correctly? Is it a truly } standardless method? What precautions should be taken? } } 2. I checked a EuS sample. I used Eu L lines and S K line. It gives } about 70%Eu and 30%S, which is way off the stoicheometric value. The } sample is believed to be not far from 50%Eu and 50%S. } The result of a GaAs sample seems reasonable. } So what is the reason for this result? because of using L lines? } } I would appreciate very much help and suggestions on this. } } Regards } Yan Xin
** Anthony J. Garratt-Reed ** MIT Room # 13-1027 ** 77 Massachusetts Avenue ** Cambridge, MA 02139-4307 ** USA ** ** Phone: (+) 1-617-253-4622 ** Fax: (+) 1-617-258-6478 **
As you probably know, Ladd is the world's largest producer of burr-free apertures for both EM's and a wide variety of other applications. The question of moly vs. platinum has come up quite often over the past 50 years. It all boils down to customer preference.
Some points: 1. The cost for both is the same. 2. Some users feel moly being harder will last longer. 3. Platinum can be flamed, moly requires an evaporator.
Since a single hole aperture is quite inexpensive and lasts a long time in a modern EM they tend to become disposable after one or two cleanings. So we suggest platinum. Just pull it out, flame it and put it back in.
Multi-hole strips are more expensive and evaporator cleaning will lengthen the life so moly might be the best choice. Some strips and plates we do have 20 or more holes.
Based on our experience we have the following general recommendations: single hole EM disc - platinum multi-hole plate or strip - moly X-ray plates or discs - tantalum satellites - stainless steel ION beam - moly infrared - stainless steel
Disclaimer: Ladd sells EM supplies and accessories
John Arnott Ladd Research 83 Holly Court Williston, VT 05495
On-line Catalog: http://www.laddresearch.com
tel: 1-802-658-4961(anywhere) or 1-800-451-3406(US) fax: 1-802-660-8859 e-mail: sales-at-laddresearch.com ----- Original Message ----- } From: "Kestutis Smalinskas" {smalinskas-at-yahoo.com} To: {Microscopy-at-sparc5.microscopy.com} Sent: Friday, September 27, 2002 11:11 AM
What do you mean by "it gives about 70% ...."? Is it something the computer spits out when you click composition analysis? Hope it is not.
A 'correct' quantitative composition analysis requires a reasonable solid background on what EDS is about. A book by goldstein (SEM and X-ray microanalysis) covers reasonable background on this topic.
There are artifacts and complications. To mention some: silicon x-ray escape peaks, silicon fluorescense, sum peaks... these are probably not taken into consideration by the computer in 'spitting' the final composition. Tilt angle (detector-sample), homogeneity of samples, absorption, are some of other things you should take into consideration when doing a 'more precise' quantification.
Cliff-Lorimer constants can give some idea about relative composition for different elements. However, to do a reasonable 'correct' quantification, I will definitely suggest a standard with known composition.
DTSA is a program that allow data manipulation (such as background substraction), and simulating different parameters (such as angle, etc). It's free, but works only on Mac.
Alternatives are using other method to do composition measurement. There are other methods that give a (much) better accuracy than EDS in TEM, unless you are looking at a small feature in your sample.
Edy Widjaja Materials Science and Engineering Northwestern University reply to : e-widjaja-at-northwestern.edu office : 847-491-7809 lab : 847-491-3281 http://www.numis.nwu.edu/internet/Staff/edy
On Fri, 27 Sep 2002, Yan Xin wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Dear listers, } } I have some questions concerning quantitative composition analysis by EDS } in a TEM. } 1. how do I do the quantitative analysis correctly? Is it a truly } standardless method? What precautions should be taken? } } 2. I checked a EuS sample. I used Eu L lines and S K line. It gives about } 70%Eu and 30%S, which is way off the stoicheometric value. The sample is } believed to be not far from 50%Eu and 50%S. } The result of a GaAs sample seems reasonable. } So what is the reason for this result? because of using L lines? } } I would appreciate very much help and suggestions on this. } } Regards } Yan Xin } ======================================= } Yan Xin (Ph.D) } Magnet Science & Technology } National High Magnetic Field Laboratory } Florida State University } 1800 E. Paul Dirac Drive } Tallahassee, FL 32310 } Tel: (850) 644 1529 } Fax: (850) 644 0867 } ======================================== } } } } }
Stu Smalinskas wrote: ==================================================== I notice in some catalogs, that one has the option of ordering either Platinum or Molybdenum apertures. what are the advantages and disadvantages between the two? ==================================================== This is one of our most frequently asked questions and we have tried to cover it on our URL http://www.2spi.com/catalog/apt/aptintro.html
Disclaimer: SPI Supplies has offered both platinum and moly apertures for some number of years to our customers in the electron microscopy world. Our vested interest is making sure our customers gets what is best from their applications standpoint.
Chuck
PS: Remember that we are striving to be 100% paperless, therefore there are no paper copies kept of this correspondence. Please be sure to always reply by way of "reply" on your software so that the entire string of correspondence can be kept in one place. ============================================
Charles A. Garber, Ph. D. Ph: 1-610-436-5400 President 1-800-2424-SPI SPI SUPPLIES FAX: 1-610-436-5755 PO BOX 656 e-mail:cgarber-at-2spi.com West Chester, PA 19381-0656 USA Cust.Service: spi2spi-at-2spi.com
Look for us! ######################## WWW: http://www.2spi.com ######################## ============================================
on 9/27/02 9:56 AM, Yan Xin at xin-at-magnet.fsu.edu wrote:
} } I have some questions concerning quantitative composition analysis by EDS } in a TEM. } 1. how do I do the quantitative analysis correctly? Is it a truly } standardless method? What precautions should be taken? } } 2. I checked a EuS sample. I used Eu L lines and S K line. It gives about } 70%Eu and 30%S, which is way off the stoicheometric value. The sample is } believed to be not far from 50%Eu and 50%S. } The result of a GaAs sample seems reasonable. } So what is the reason for this result? because of using L lines? } } I would appreciate very much help and suggestions on this. } Dear Yan Xin, 1) There are standardless methods, which depend on theoretical calculations. When last I looked, these calculations were somewhat uncertain, although they may have improved. If you have standards for Eu and S in a matrix that is as close as possible to that of the sample you are examining, you can check whether the standardless analysis matches your standards. 2) I suspect that the S may be volatile, but I may be way off base. If you are using the correct parameters for production of the Eu L line, the calculation should be correct, so use of the L line should not be the reason for the result. If, however, your standardless analysis program automatically inserts the parameters for K lines without giving you a choice, this will obviously lead to an error. Yours, Bill Tivol
I am a young researcher on materials and transimission electron microscopy for 10 years(5 patents, 15 papers including 1 paper in one of the best journals and some in famous SCI journals). I am hunting a reseach position (or post-doctoral postion). If someone has such a position and is interested in me, keep in touch with me.
Thank you very much
Yours sincerely
Gao Yihua ---------------------------------------------------------------------------- Dr. Yihua Gao (Y.H. Gao) Advanced Materials Laboratory and Nanomaterials Laboratory, National Institute for Materials Science, Namiki 1-1, Tsukuba, Ibaraki 305-0044, Japan Email: GAO.Yihua-at-nims.go.jp; gaoyihua-at-yahoo.com TEL: 81-298-513354(ext.662) Fax: 81-298-516280 ----------------------------------------------------------------------------
Thanks for your answers. I probably should have mentioned that I clean my apertures mechanically. If you remember, I'm the one that posted about using 1 to 6 micron diamond and metallographic cloth to polish apertures, so baking under vacuum (or without vacuum) is not an issue.
Stu Smalinskas Metallurgist SKF NATC Plymouth, Michigan
__________________________________________________ Do you Yahoo!? New DSL Internet Access from SBC & Yahoo! http://sbc.yahoo.com
Best bet is dump the diamond paste and use regular polishing compound on moly apertures. Moly's hardness along with the softer polish will assure a long life for the apertures. Regular cotton twill lint-free cloths or Kimwipes work well for polishing.
Here's another clue, one I haven't shared with folks here yet. I spent years looking for a simple compound for cleaning optics parts that I could take to customer labs and use without worry about their many different environmental concerns. I found it a couple of years ago and have been using it with good success. As far as I am aware, there are no restrictions or serious cautions on its use or disposal.
The compound is Sodium Metasilicate, a popular replacement for TSP based wall cleaners that's available in just about every hardware store. I've used a mild (a couple of grams to 500mL water, nothing exact) solution to ultrasound the parts in. It takes a while, 20 - 30 minutes, but gets rid of most of the contamination on its own. What remains is a lot easier to remove with light polishing. Polished brass parts come out bright. The package will caution about a mild etching action on polished aluminum and glass - I've haven't noticed it on either, but it is probably because of the dilute concentrations I use. Other materials seem unaffected. Perhaps higher concentrations would clean better on parts not affected by the etching.
Another nice feature is using water (DI or distilled) as the solvent for steps that use large amounts of solvents - tends to make you rinse things better. Any parts needing polishing I then ultrasound in the solution again to remove the particulates. All parts get well rinsed with water and a careful hand rinse with a squirt bottle of methanol, ethanol, isopropyl or acetone to remove any remaining water prior to reinstallation.
In this case, it will help the apertures last longer. In fact, if you clean them more frequently, you might find that the solution itself will be sufficient and you won't need to polish them.
If anyone uses this, let me know how it works for you.
Allen R. Sampson Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174
On Saturday, September 28, 2002 3:15 PM, Kestutis Smalinskas [SMTP:smalinskas-at-yahoo.com] wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Thanks for your answers. I probably should have } mentioned that I clean my apertures mechanically. If } you remember, I'm the one that posted about using 1 to } 6 micron diamond and metallographic cloth to polish } apertures, so baking under vacuum (or without vacuum) } is not an issue. } } Stu Smalinskas } Metallurgist } SKF NATC } Plymouth, Michigan } } __________________________________________________ } Do you Yahoo!? } New DSL Internet Access from SBC & Yahoo! } http://sbc.yahoo.com } } }
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Just some additional thoughts on material choice for apertures:
When you speak of a Pt aperture it is probably Pt/Ir. The iridium allows for easier machining. We do pure platinum and gold apertures but only when the application demands it.
Another important consideration is the number and sizes of a multi-hole strip or plate. We have put up to 30 holes, some as small as 1micron, in a single part. Since the manufacture of burr-free, concentric apertures requires that the holes be made individually, more holes and smaller sizes result in more material losses during production. Platinum costs can add up.
For ultra-small holes and multi-hole parts moly should be used whenever possible.
John Arnott Ladd Research 83 Holly Court Williston, VT 05495
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} Please send resumes and direct inquiries to: rccieslinski-at-dow.com } } POSITION OPEN } } Polymer Electron Microscopist } The Dow Chemical Company } Midland, Michigan } } Dow’s Corporate R&D Analytical Science Laboratory has a professional level } opening for a polymer microscopist at it’s Midland Michigan location. The } primary responsibilities would be to design, conduct and interpret } electron microscopy experiments to provide key answers to questions } relating to the development, processing and the performance of various } materials. Good written and oral communication skills are essential. The } ability to work both independently and in a team environment is also } extremely important. } } Educational Requirements: } A Ph.D. or MS degree in a materials or chemical related discipline is } preferred, but candidates with in a biological science related discipline } and substantial materials EM work experience would be considered. } } Experience Requirements: } Experience operation of a transmission electron microscope; excellent } manual dexterity and visual acuity; demonstrated ability to acquire and } objectively interpret data, and hands-on experience in the preparation of } specimens for Electron Microscopy, including ultramicrotomy and } cryo-ultramicrotomy. } } Key responsibilities will include: } * Strong problem solving skills. } * Active participation in development and project work teams. } * Interpretation and documentation of work } * Compliance with safety and quality programs. } } Send resumes and direct inquires to: rccieslinski-at-dow.com } } Robert C. Cieslinski, Ph.D. } The Dow Chemical Company } Corporate R&D, Analytical Sciences } 1897E Bldg. } Midland, MI 48667 } Fax: (989) 638-6443 } Email: rccieslinski-at-dow.com } } The Dow Chemical Company is the second largest chemical company in the } world and a leader in science and technology solutions. Come visit Dow } careers on the web at http://www.dow.com/careers. }
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