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The answer to this very much depends on what you are charging for. To find an answer, you need to identify (a) the net costs you wish to recover: e.g. capital costs (to be recovered over what period?, at what rate of interest?), running costs, salaries of direct (em technician) and indirect (clerical, admin.) support staff including overheads, any charges for space occupancy and services etc., less any subsidies (b) make a realistic estimate of the maximum number of hours per year that a charge can be recovered from. The answer is a/b. Simple, isn't it? Well, no. In practise you will probably find that b is dependent on a/b since all categories of users are sensitive to price, but you will have to model this differently for different categories of users.
Our charges per hour for self-help access to a Philips CM120 Biotwin are as follows: Departmental £15, Other departments £21, other publicly-funded research organisations £35, industrial £70. Non-attenders incur full charge for the period booked. These numbers were not exactly arrived at using rocket science. We charge extra for all materials consumed (film, processing) and for direct user-support from a technician. We do not include capital costs recovery in our charges.
I would strongly advise imposing a special concessionary charge on users who insist on tipping their specimens and retaining circlips into the guts of the Compustage! An electronically-operated trap door beneath the operator's seat is also an attractive option.
Chris
} From: "Ping Li" {pli-at-is.dal.ca} To: {Microscopy-at-sparc5.microscopy.com}
Folks: A Happy New Year to you all I thought I should let you all know about the Third annual course in Quantitative Fluorescence Microscopy to be taught between june 17 and 22th 2001 at the Mount Desert Island Marine Biology Laboratories in Arcadia National Park in Maine. This team taught course led by Dave Piston (Vanderbilt), Mike Nathanson (Yale), Guillermo Romero (Pittsburgh) and myself focusses specifically on the development and application of modern fluorescence microscopic methods. This six day intensive course covers all aspects of the technology from microscope and dye design, cameras, confocal microscopy, live cell microscopy, multiphoton microscopy and GFP. Considerable attention is also given to quantitative analysis in 2 and 3 dimensions and time. The specific focus of the course allows an in depth treatment of these methods. The goal of the course it to teach students how to best implement these methods within their labs, using either their own cells and tissues or using material supplied by the course. An extensive array instrumentation, provided by all the major microscope and associated software, hardware and camera manufacturers will be available for students to use. For the last two years it has been a very successful event and so we have decided to give the course again. A full description of the course lectures together with lecture outlines, registration etc. is available at http://sbic6.sbic.pitt.edu/microscopy/ I would encourage you to spread the word, or sign up if you are interested. The total number of students is limited to 25, enrollment is decided by the course faculty. If you have any further questions please feel free to contact me Thanks Simon
--------------------------- Simon C. Watkins Ph.D. MRC Path Associate Professor, Cell Biology and Physiology Director: Center for Biologic Imaging BSTS 225 University of Pittsburgh Pittsburgh PA 15261 Tel:412-648-3051 Fax:412-648-8330 http://sbic6.sbic.pitt.edu -----------------------------------
} There is a position for an EM technician at the Electron } Microscopy Core lab of the Biotechnology Program at the University of } Florida in Gainesville. The laboratory is mostly a fee-for-service lab } serving the needs of biological, biomedical and agricultural scientists } at the university. Applicants must be skilled in the preparation of } biological samples for both scanning and transmission electron } microscopy. Experience with both PC and Mac as well as website } management is desirable. Experience with digital imaging and } fluorescence microscopy also a plus. } This is a full time, permanent position with standard benefits of } State of Florida employees. } } For further details, reply to this message or contact Greg Erdos } at the number below. } } }
Gregory W. Erdos, Ph.D. Assistant Director, Biotechnology Program PO Box 110580 University of Florida Gainesville, FL 32611
As part of the planned makeover of our building, it has been proposed that the various and somewhat distributed microscopy facilities in our building - SEM, TEM, Confocal, fluorescence, luminescence imaging, darkroom etc. etc. might be brought together to form a biological imaging facility, thereby benefitting from some improvements in supervision, security and user support. Part of that proposal was to set up a computing lab with fileserver and work- stations networked to the instruments and dedicated to image storage and off-line image and spectral processing and analysis. However, there is great pressure on space in this building, and it has been suggested to me that computing for imaging and spectroscopy does not need to be separated from general purpose computing these days. What are your opinions about this? Pro or con?
Happy New Millennium Chris ~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~ Dr Chris Jeffree University of Edinburgh Biological Sciences EM Facility Daniel Rutherford Building King's Buildings EDINBURGH EH9 3JH Tel: +44 (0) 131 650 5345 FAX: +44 (0) 131 650 6563
Hi Tim, I like your idea of a separate step for the UA*. Though 1% may be overkill. We routinely use a cocktail for freeze-sub consisting of: 1) 4% osmium tetroxide in HPLC grade acetone 2) 0.1% uranyl acetate also made with HPLC grade acetone - make this up the day before the freezing so it has time to go into solution before chilling. Mix together 1:1 for wonderful contrast. *We have to use Radiation Safety Services for disposal of this cocktail because our hazardous waste folks refuse to deal with the combination of OsO4 and UA.
Another angle - You didn't mention the type of resin you're using. Freeze-sub tissue is often murky looking (low contrast) when it is embedded in 100% Spurr's. We use Araldite/Embed 812 (an EMS kit) or a mixture of equal parts Spurr's and Araldite/Embed 812.
hope this helps, Beth
} Hello Out There: } } I am currently involved with a cryo substitution project with human red } blood cells. I have replaced the non crystalline ice with 2% Osmium in 100% } acetone and have OK morphology, but the contrast is a bit low. I am } thinking about trying to follow the Osmium step with uranyl acetate, before } embedding in plastic. Does any one out there know if 1%uranly acetate will } be OK in 100% acetone? Thanks, Tim } } Timothy G. Schneider } Director of Electron Microscopy } Department of Pathology } Room 229 Jefferson Hall } Thomas Jefferson University } 1020 Locust St. } Philadelphia Pa. 19107 } 215-503-4798 work } 610-613-8170 cellular } timothy.schneider-at-mail.tju.edu
************************************** Beth Richardson EM Lab Coordinator Botany Department University of Georgia Athens, GA 30602
I use Ralph type glass knives for plastic sectioning of biological samples. I am experiencing problems in making a proper knife. I have a TAAB histoknifemaker (also says Reichart-Jung). Is there anyone willing to offer expertise in this area?
Within the last couple of days (and, therefore, not in the recently posted archives) someone posted a note about a used chiller that they had for sale. I've lost the note. If still available, could you please repeat the note to my email address: edsworth-at-aol.com Thanks.
Ed Holdsworth General Mgr. SEMTEC Laboratories, Inc.
Those of you who need to process electron diffraction ring patterns (recorded from thin polycrystalline or amorphous samples in a TEM) might be interested in the FREE program (for IBM PC, Windows op. system) that can be downloaded from my home page (below). The program produces XRD-like output from digitized SAED ring-patterns and compares to markers showing the positions and intensities of known phases. The newest version (1.2.0) of this ProcessDiffraction program provides easier operation and new functionality:
* Built-in hints: what to do next (and how). Can be switched off.
* File-name and path can be specified for output. Default paths are suggested separately for input SAED, input Marker and output. Manually selected paths can be stored as default (during exit).
* No limit on BMP file-size.
* The automatic peak-list can be manually extended using Cursor.
* Selection of individual points (in the SAED for reading-out of d-value and establishing correlation between distribution and SAED) is aided with a Cursor with increased contrast and magnification.
* Units of X-axis can be changed to the physically meaningful scattering vector [1/A] (in contrast to pixels).
* Several net distributions can be compared
* Individual markers have different colors.
* Renormalized Gross intensity can be calculated by excluding pixels with zero intensity (i.e. corresponding to beam-blocking pin) from the averaging process.
* Renormalized Net intensity can be calculated. Here points with intensity above the average (over a given circle) are only included in the averaging. Average intensity of bright pixels within a discontinous ring are only calculated this way, giving more realistic intensity of a diffraction line for comparison purposes.
* Show menu is included to select which curves to show in the graph.
* Possibility to cancel is introduced at several operations.
* Automatic (fast) refinement of centre is included. In dubious cases manual selection of peak and valley is asked for.
* Calculation is double precision (basis of later extension of the software for input files with several bytes/pixel).
* Several error conditions are eliminated (crop, conflicting user requests, ..)
I hope you will like the modifications and find this program useful and easy to use. Download FREE as before from the same site.
I would appreciate having your comments and/or suggestions. Best regards:
Dr. Janos L. Labar Research Institute for Technical Physics and Materials Science H-1121 Budapest, Konkoly-Thege u. 29-33 Postal address: H-1525 Budapest-114, Po Box 49 Tel: (36)(1) 392-26-92 Fax: (36)(1) 275-49-96 Fax/phone: (36)(1) 395-92-32 home page: www.mfa.kfki.hu/~labar
University of Connecticut Institute for Materials Science
Postdoctoral Position in Electron Microscopy
The Institute for Materials Science (IMS) at UConn is an interdisciplinary center with the threefold mission of fostering education, research and outreach in all areas of the materials sciences. The Institute has a vacancy in the EM laboratory for postdoctoral researcher to work on a DARPA-funded program on Ni-based superalloys and a variety of smaller industrial projects. Candidates should hold a PhD in Materials Science, Physics or a related discipline and must have extensive hands-on experience in a broad range of electron microscopy techniques. A candidate with experience in the microstructural analysis of Ni-based superalloys using SEM and TEM would be preferred. The appointment is for one year in the first instance and is available immediately. Screening of the applications will begin immediately and will continue until the post is filled. Applications from under-represented groups, including minorities, women and people with disabilities are encouraged.
Interested candidates should send a curriculum vitae, including publication list, and the names of at least three referees with postal addresses, telephone numbers and Email addresses to: Prof. M. Aindow, Institute for Materials Science, University of Connecticut, 97 North Eagleville Road, U-3136, Storrs, CT 06269-3136 USA. Email: m.aindow-at-uconn.edu
We are a clinical diagnostic TEM laboratory serving a provincial network of hospitals. We would like to move away from conventional darkroom printing of images and wish to convert negatives to digital files. We are looking for a negative scanner that will:
1. Accept 3 X 4 1/4 inch sheet film negatives (Kodak 4489 film).
2. Comes with software support that is adaptable to a Windows format.
3. Must be priced under $3000.
4. Must provide the best quality resolution for diagnostic results (i.e. 3200 X 3600 pixel; wide linear dynamic range).
I look forward to any information and advice you can provide.
My problem is a poor knife edge. The knife looks fine under casual observation, or with small magnification, but when it comes time to actually do some sectioning, I get a lot of chattering, or streaking, or both. I know make as many test blocks as I do sample blocks, so I don't waste samples with all the bad glass knifes. I've gone through several boxes of glass over the past two months, and only get a useable knife every 15 to 20 breaks. The same knife breaker has worked fine in the past, and I have changed the scoring wheel, and checked all that I can.
This knife breaker is also very hard to get parts for. The only obvious problem is that one of the pressure points has a rubber pad that is unevenly worn. I don't see how that would cause my problem. Again, the knifes look good to the naked eye.
The glass I use is from Electron Microscopy Sciences. They are called ultra glass knife strips 6.5mm x 25mm x 400 mm.
I guess I'm just looking for someone who has had a similar problem, and fixed it in some manner. Could I have gotten a bad batch of glass? I don't think it is very likely, I've used several boxes, but they may all be from the same batch, for all I know. Is there another brand of glass, or breaker that others have found produce reliable knives?
Thanks for any and all help
-Patrick Brownell } ---------- } From: Katja M. Wolski[SMTP:kwolski-at-hsc.usf.edu] } Reply To: kwolski-at-hsc.usf.edu } Sent: Wednesday, January 03, 2001 4:26 AM } To: Brownell, Patrick } Subject: Re: Ralph Glass Knife problems } } I use a different knife machine, but what's the problem you're having? } Are you } not getting a good knife edge or what? } } Katja } } } } "Brownell, Patrick" 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 use Ralph type glass knives for plastic sectioning of biological } samples. } } I am experiencing problems in making a proper knife. I have a TAAB } } histoknifemaker (also says Reichart-Jung). Is there anyone willing to } offer } } expertise in this area? } } } } -Patrick Brownell }
I recently acquired a Zeiss OPMI with floor stand. I inspected the bulb superficially before turning it on and it seemed OK, and I confirmed the voltage was in range beforehand. However, as soon as I applied power, the filament left the prongs and the bulb was dead.
It was a Zeiss 390158 bulb, a 6v 30w triangular bayonet. It's quite possible the bulb was mechanically shocked before I got it. Was this a not unusual failure, or is there some kind of warm-up procedure that might've saved it?
A hunt through my junk boxes fortunately turned up a replacement, and it worked straight-away, even though it looks like one of the spring-like wires worked its way off the filament prongs, where the filament meets the prong wire.
For the day that this one dies, though, I'd also like recommendations for a place to purchase a replacement.
Greetings. Can anyone suggest a good all around sputter coater for general SEM use? I usually use 50 Angstrom Pt, or Carbon for EDS. Thanks in advance.
Tracy E. Anderson Microscopy Specialist Surface Characterization Dept. SurModics, Inc. www.surmodics.com tanderson-at-surmodics.com
Anyone else happen to watch "Mysterious Ways" earlier this week. One character was chatting with another about the fantastic new TEM they were using with the "Kevex EDS system with the twin Quantum 10-mm2 detectors". I had to listen quick to hear it.
Granted, its a bit dated (Thermo-Noran is now the name and they don't list the Quantum on their web page), and some of their other references to other techniques were of questionable accuracy. Still, I was tickled to see a reference to EM on TV. I remember a few references on "Quincy", but not a lot since.
Disclaimer - I don't have a twin Quantum system, but am still using a 10-mm2 Quantum on our JEOL-840.
Hi all: Can anyone tell me who the current manufactures of ultra microtomes are? -- Regards, Gregory Rudomen Technical Specialist Electron Microscopy State University of New York at Stony Brook University Microscopy Imaging Center Stony Brook, NY 11794-8088 631-444-7372 Greg-at-umic.sunysb.edu ************************************************* Standard disclaimer: The opinions expressed in this communication are my own and do not necessarily reflect those of the University Microscopy Imaging Center. *************************************************
Bulbs of the most exotic sort can be found at: 1. Bulbtronics;(516)-249-2272 2. Bulb Direct; 1-800-772-5267, or info-at-bulbdrect.com
Good luck,
Sam Purdy Technical Center, National Steel Corp. Trenton MI 48183 Voice; 734-676-2682 FAX 734-676-2030 E-mail spurdy-at-nationalsteel.com } ---------- } From: John Foust } Sent: Wednesday, January 2001, 11:49 AM } To: Microscopy-at-sparc5.microscopy.com } Subject: Zeiss lamp failure question } } ------------------------------------------------------------------------ } 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 recently acquired a Zeiss OPMI with floor stand. } I inspected the bulb superficially before turning } it on and it seemed OK, and I confirmed the voltage } was in range beforehand. However, as soon as I } applied power, the filament left the prongs and } the bulb was dead. } } It was a Zeiss 390158 bulb, a 6v 30w triangular } bayonet. It's quite possible the bulb was } mechanically shocked before I got it. Was this } a not unusual failure, or is there some kind of } warm-up procedure that might've saved it? } } A hunt through my junk boxes fortunately turned up } a replacement, and it worked straight-away, even though } it looks like one of the spring-like wires worked its } way off the filament prongs, where the filament meets } the prong wire. } } For the day that this one dies, though, I'd also like } recommendations for a place to purchase a replacement. } } - John } }
Tracey E. Anderson wrote: ====================================================== Greetings. Can anyone suggest a good all around sputter coater for general SEM use? I usually use 50 Angstrom Pt, or Carbon for EDS. Thanks in advance. ====================================================== SPI Supplies manufactures a modular coater that is robust, requires little maintenance, and will do all of the precious group metals, including Pt. Carbon is done via the carbon coater module. A number of other firms manufacture sputter coaters for SEM applications and they can all be found on the following two vendor data bases:
Microscopy Vendor's Data Base http://207.137.96.185/mvd/vendors.html
MicroWorld Resources and News http://www.mwrn.com/
Disclaimer: SPI Supplies manufactures sputter and carbon coaters for SEM laboratory applications.
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 ############################ ==================================================
MAS membership renewal application forms were mailed late last week. Enclosed with your application is the 2000 Membership Directory. Please make any corrections on your form and return it along with your dues in the envelope provided. My sincere apology for the late mailing.
If you have any questions, do not receive your renewal packet, or are not a member of MAS and would like to join, please contact me either at work or at:
MAS Membership Services PMB 141 2101 W. Broadway Columbia, MO 65203-1261 1 (800) 4MASMEM masmembership-at-excite.com
Thanks, Lou Ross Senior Electron Microscope Specialist Electron Microscopy Core Facility W136 Veterinary Medicine University of Missouri Columbia, MO 65211 (573) 882-4777, fax 884=5414 email: rosslm-at-missouri.edu web: www.missouri.edu/~geosclmr/ebaf.html
Vitaly Feingold Scientific Instruments and Applications 2773 Heath Lane, Duluth GA 30096 (770)232-7785 ph. (770)232-1791 fax
This message is made of 100% recycled electrons. -----Original Message----- } From: John Foust {jfoust-at-threedee.com} To: Microscopy-at-sparc5.microscopy.com {Microscopy-at-sparc5.microscopy.com}
What constitutes a "good all around" sputter coater is perhaps somewhat vague? If you are looking for something that is easy to use and provides consistent results, that may be a problem.
New units are in the $4K to $8K price range. This depends on whether it has a pump included, thickness measuring unit (not all that usefull, IMO) and type of target, and dual mode or single plating mode. These units are sputter coaters, not evaporation units.
I searched for what it sounds like you are doing the same. I narrowed the search to a Denton Desk II or an Anatech Hummer VII. I settled on a used Hummer. This is an obsoleted unit. But after some initial hickups, this coater works really well. Everything is contained in one unit. It has old metal gate CMOS digital ICs (still available) and an Edwards or Alcatel small pump inside. It will do etching and plating. What I like about this unit is that it will do plating at a specified rate with a specified end point thickness. These settings must be validated to be absolutely correct. The rate and power can be adjusted via pots to hone the correlation of settings and results.
Newer units cost tons of money and do not do a proportionately better job. They are basically manual units. Set the time, and make the run. No idea of thickness. Pump is optional...right. Thickness measurement options are a waste of money in my opinion. The results are not repeatable. And the most common measuring method is a quartz crystal. This is a consumable item.
You have a tough decision, based on my experience. I would suggest that you look for a used Hummer VII or a Desk II. I just don't think that the newer units are all that great of a value. Nor are they all that user friendly. But YMMV.
gary g.
At 12:44 PM 1/3/01, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
I am participating in an art project that incorporates micro-organisms (e.g. euglena although larger ones e.g. hydra are feasible) as actors. The video from the microscopes/cameras will be streamed in realtime via the Internet.
Image quality is important to us, cost less so although there shall be several stations in different geographical locations.
Should one wish to suggest a particular microscope and camera we would be delighted. (The software isn't an issue)
A European company -Digital Biomedical Imaging Systems AG (DITABIS), produce a plate scanning system that may suit your future needs, but I'm not certain whether you can scan negatives with it. It's an imaging system to replace using negatives; I don't know if they have a distributor State-side but a while back I made contact with a British company at the Micro 2000 conference, UK, who are distributors for the system in the UK and they were willing to let customers have a trial run with the scanning plates.
A web site http://www.ditabis.de/first.html explains the system
The UK company is
ISS group services Pellowe House Francis Rd Withington Manchester M20 9XP
Phone:+44 161 445 5442 Fax:+4 161 445 4914
They don't appear to have a web site
Hope this info is of some use + I stress that I have absolutely no commercial or other interests with the above companies.
Mr. Cameron Hind Research Scientist Advanced Technologies group Baxter R & D Europe S.C.R.L. Rue du Progrès 7 1400 Nivelles Belgium
Hi John In reference to your request for replacement bulb 39-01-58...I currently use Bulb Direct for all my lighting needs. 1-800-772-5267 WWW.BULBDIRECT.COM This company is very good on delivery (2 days) and have the best prices I have run across.
I have no affiliation with Bulb Direct just satisfied customer.
Can anyone advise me on what chemical sample I can use to test the (in)accuracy of EELS quantification for oxygen. Is there an oxide for which there is abselutely no doubt on the oxygen concentration. Preferably with a metal which has a good EELS peak (below 1 keV). The goal is to have a reference with a reliable metal/O ratio.
Facility Manager Position Electron Probe Instrumentation Center Northwestern University
The Electron Probe Instrumentation Center (EPIC) at Northwestern University has an immediate opening for a full-time facility manager to assume the responsibility of managing the advanced EM laboratory and facilitate/initiate advanced TEM research. Responsibilities also include supervision of two technical staff in SEM and specimen preparation. The EPIC facility serves over 100 users in all aspects of Scanning and Transmission electron microscopy. The role of the Facility Manager is to provide leadership in advanced electron microscopy in materials research, and assist users with their advanced TEM needs, including the following: teaching/assistance in: HRTEM, nanodiffraction, EDS, EELS, image processing, etc. A strong laboratory development component, research initiatives and commitment to teaching are associated with this position. All EMs in EPIC are under full service contract. Thus, the duties include mainly training students/users in their research needs, development of specialized techniques and applications for materials research, and minor records and fiscal management. A PhD in physical sciences/engineering is required. The candidate must have hands-on experience in all aspects of advanced TEM as well as digital acquisition, processing and computer assisted techniques. All levels of experience will be considered. Compensation commensurate with experience and qualifications. Promotion to research faculty position is possible with proven research credentials. Send cover letter, resume and three references to: Prof. Vinayak P. Dravid, Director EPIC Materials Science & Engineering Northwestern University, 3013A MLSB Evanston, IL 60208 E-mail: v-dravid-at-northwestern.edu Fax: (847) 491-7820 http://epic.ms.nwu.edu/epic/index.htm
Northwestern University is an Affirmative Action/Equal Opportunity Employer. Hiring is contingent upon eligibility to work in the United States.
I am a research assistant at Catholic University and have been attempting for the past few months to thin section alteration layers, (in cross section,) of simulated nuclear waste glasses subjected to vapor hydration testing. These altered layers are typically comprised of multiple phases, frequently composed of various alumino-silicates, and are brittle and porous. They range from a few microns to hundreds of microns. When fragmented off the test coupon, usually a few microns (~1-20um) of glass remain adhered to altered region. We are interested in this transition region between the glass and altered layers.
Dozens of attempts have been made to section these materials once embedded. Variations of impregnation protocols have been tried with recipe variations utilizing Spurr’s resin. Block faces on average have been ~200x500um with particles sizes anywhere from a few microns to ~200um. Utilizing a Sorvel MT-2, cutting speeds between 0.25 and 2.5mm/second have been attempted, (the full range of the instrument.) The diamond knife is new. The advance has been altered between 20nm and 250nm – producing the appropriate interference colors, but with voided regions wherever the particles are situated. I have tried everything I could think of to facilitate infiltration/adhesion of these particles within the embedment medium. After thousands of sections from 80+ blocks and several protocols, I haven’t had the slightest glimmer of success. I know the very thing we have been attempting has been successfully done at ANL. So, I implore anybody that has any specific insight, simple thoughts, or longshots to let me know.
Sincerely,
Cavin T. F. Mooers Research Assistant The Catholic University of America 434 Hannan Hall Washington, D.C. 20064 (202) 319-5346 phn (202) 319-4469 fax
And now, from the Last Hope Department, I was wondering if anyone out there has an old Leitz Tas Plus Image Analyzer? This would be of mid-'80's vintage, comprised of a bench with a pop-up monitor with light pen, a nice microscope with built-in video capability, and a big black electronics box about four feet tall (containing 2 8-inch floppy drives - like I said, this thing is old). Long story short, ours is broken, and we can't even begin to fix it without schematics (some clever soul -no, not me - tossed them out years ago). If anyone happens to have a set of the electronics schematics for one of these things hanging around, please contact me ....we'll talk....
Frank Thomas MicroAnalysis Facility Geological Survey of Canada (Atlantic) P.O. Box 1006 Dartmouth, Nova Scotia Canada B2Y 4A2
Gatan, Inc., the technology leader in digital imaging, analytical spectroscopy and icon beam milling applications for electron microscopy in Pleasanton, CA., is seeking candidates for a TEM Laboratory Manager. This person will manage the TEM applications laboratory. Responsibilities include coordinating all activities related to customer demonstrations and training, Applications material generation and supporting the R&D department utilization of the TEM systems. Some travel within and outside the USA is required. Applicants should have significant TEM and CCD imaging experience. Biological, materials or semiconductor experience would be useful. Familiarity with existing vendors, consultants, competitors, etc in the industry is a plus. Knowledge of Gatan's software and hardware applications. A proven track record in both planning and managing a laboratory environment and outstanding computer/PC skills. Must be comfortable with current development environments and development tools to work intelligently with engineering. Must have excellent overall PC computing skills, including a thorough familiarity with market tools in document composition, database design and presentation management. PhD, desired; technical background preferred. Salary: Base salary plus bonus commensurate with experience.
Interested candidates should send, email or fax their resume to:
GATAN, INC Attn: HR Department 5933 Coronado Lane Pleasanton, CA. 94588 Fax: (925) 463-0204 Email: hr-at-gatan.com www.gatan.com Carlotta Daniels GATAN, Inc. Human Resources
Calvin, Hard materials such as glass can be readily microtomed with a diamond knife (even diamond coated silicon in Microscopy Research and Technique, vol. 31, p. 308, 1995). Any good diamond knife will work with meticulous and careful technique, but experience has shown that 35 degree knives yield the best results with hard and ultra-hard materials.
It sounds as though your samples may be large and adhesion to the epoxy is poor. In order to microtome non-porous materials such as glass, you should first minimize the cross-sectional area to be sectioned. An easy way is to do this is to pop concoidal micro-chips from the surface. These tend to be very thin at the edges and can be further broken to form pointed thin samples. Another critical element is to improve adhesion of the sample to the resin (Spurrs) with the use of an adhesion promoter such as Dow Corning Z-6040. Submerging the sample in a 2% solution of Z-6040 (50/50 ethanol and H2O) for 30 minutes allows a surface reaction that promotes adhesion of glass to epoxy. Remove samples from the solution, air dry, and embed in Spurrs. Then, microtome using standard procedures with sectioning speed reduced to 0.1 mm/s.
Cheers,
Phil Swab, Sr. Engineer Engineering Development Group Deposition Sciences, Inc 386 Tesconi Court Santa Rosa, CA 95401
-----Original Message----- } From: Cavin Mooers [SMTP:cavinm-at-vsl.cua.edu] Sent: Thursday, January 04, 2001 6:30 AM To: Microscopy-at-sparc5.microscopy.com
Dear Microscopists,
I am a research assistant at Catholic University and have been attempting for the past few months to thin section alteration layers, (in cross section,) of simulated nuclear waste glasses subjected to vapor hydration testing. These altered layers are typically comprised of multiple phases, frequently composed of various alumino-silicates, and are brittle and porous. They range from a few microns to hundreds of microns. When fragmented off the test coupon, usually a few microns (~1-20um) of glass remain adhered to altered region. We are interested in this transition region between the glass and altered layers.
Dozens of attempts have been made to section these materials once embedded. Variations of impregnation protocols have been tried with recipe variations utilizing Spurr's resin. Block faces on average have been ~200x500um with particles sizes anywhere from a few microns to ~200um. Utilizing a Sorvel MT-2, cutting speeds between 0.25 and 2.5mm/second have been attempted, (the full range of the instrument.) The diamond knife is new. The advance has been altered between 20nm and 250nm - producing the appropriate interference colors, but with voided regions wherever the particles are situated. I have tried everything I could think of to facilitate infiltration/adhesion of these particles within the embedment medium. After thousands of sections from 80+ blocks and several protocols, I haven't had the slightest glimmer of success. I know the very thing we have been attempting has been successfully done at ANL. So, I implore anybody that has any specific insight, simple thoughts, or longshots to let me know.
Sincerely,
Cavin T. F. Mooers Research Assistant The Catholic University of America 434 Hannan Hall Washington, D.C. 20064 (202) 319-5346 phn (202) 319-4469 fax
Hi, we have some imaging problems with Zeiss LSM 410. Sometimes, when we collect an image series, one or more of the images had different sized lighter or darker bands across the images. This happened with both green and red channels (488 nm and 543 nm). It occurred randomly. In addition, sometimes, the image suddenly totally whited out during the scanning. In which case, the up part of the image looks normal, but the lower part is white. In all cases, there were no indication of any changes in pin hole size, contrast, brightness, and laser power based on the readings showed in the LSM program. I am not sure what is wrong. Could be the scanner? video card? or may be something else? Could any of you please help me and tell me what do you think the problems are? Any information is highly appreciated.
I am using regular EPSON Expression 1600 flatbed scanner with "transparency adapter". It has 1600 optical dpi resolution and pretty fast. To eliminate the Newton rings, you may use special cassettes to hold the film. Unfortunately, EPSON does not provide the cassettes for standard EM film. You have to made them in machine shop (not big deal, actually). I do use some EPSON cassette, which is bigger than my film in one dimension, but it works well. This scanner comes with very good software and you may scan your images directly into Photoshop or any other suitable program. I am scanning in "positive transparency", 12-bit (Hi-Fi) gray, 1600 dpi mode and than adjust the levels in the Photoshop (to remove the "empty" levels of gray), transfer in 8-bit mode and save. Usually, I prefer to keep the original 12-bit image as well, but it's huge - about 50 Mb each. I am using 2.6 or 5.2 Gb MO disks for storage.
I hope it will help.
Sergey
P.S. I have no interest in EPSON products, just happy user.
At 11:24 AM 1/3/01 -0400, 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
This equipment specially designed to work with "image plates". Nothing related to the negatives. Moreover, they claimed that their system is supposed to substitute the regular photo-process (and in some instances that works better, linearity and sensitivity, for instance). Only one disadvantage - very pricey and time consuming.
Sergey.
At 09:50 AM 1/4/01 -0600, 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
I think Phil is right. You better collect really a small smaple which is like a needdle. At the frond end of your needle, you will have the altered layer plus a little glass. Crack your corroded glass samples you can always find out a tiny needle suitable for ultramicrotomy. You may read our paper in Journal of Nuclear Materials (Vol. 254, pp. 249-265, 1998) for your reference.
Good luck,
Weiliang Gong Center for Radioactive Waste Management University of New Mexico 1001 University Blvd. Se Albuquerque, NM 87106
Hello- Does anyone out there know the scintillator sizes for the upper and lower secondary electron detectors on a Hitachi S-4500? Also, does anyone have an opinion on whether the single crystal YAP (or YAG) scintillators are worth 10x the money of a P-47? The catalogues say they last longer and have better S/N even though they produce less signal than the P-47. If I switched, would there be adjustments I would need to make to my SEM? Thanks for your help.
We are considering purchasing a Nikon Coolpix digital camera for use on light microscopes. We would like to know if anyone has experience using these cameras for fluorescent microscopy. Is the meter accurate at low light levels? Thanks.
Richard Demaree, Ph.D. Dept. Biological Sciences Calif. State Univ., Chico Chico, CA 95929-0515 530-898-5812 rdemaree-at-csuchico.edu
I am trying to find a way to perform immunofluorescence in plant protoplasts for both cytosolic and peroxisomal proteins.
My problems are as follows:
1) Fixing of the protoplasts prior to immunofluorescence is difficult; fixation in 4% paraformaldehyde, 350 mM mannitol, and 50 mM sodium phosphate, pH 7 for 50 min followed by treatment with 0.1% triton X-100 for 10 minutes yields protoplasts that appear to be aggragated and broken.
2) Fixing of protoplasts expressing cytosolic GFP, as detailed above, loose their GFP-fluorescence.
Does anyone have an established method for plant protoplast immunofluorescence?
Thanks
Kristi Snell
-- Dr. Kristi D. Snell Metabolix, Inc. Cambridge, MA
Greetings. I would like to look at a cross section of a standard sized glass slide under TEM. Does anyone know how I could prepare such a sample? Will a microtome work? Any suggestions would be very much appreciated.
Tracy E. Anderson Surface Characterization Specialist SurModics, Inc. 952.829.2720 Voice 952.829.2743 Fax tanderson-at-surmodics.com
There are a number of standard methods that will work.
Microtomy should work. There has been a recent thread about some porous glass. You should see the postings by Phil Swab. He also has a Journal article that you might be able to get a copy from Stacie Kirsch on how to do cross section of glass using microtomy. He recommends a 35 degree knife. Basically, you create small shards from the surface of the glass, mount them and then cut them. If you know how to microtme and do not know any of the other standard cross sectional preparation techniques, I would go with this one.
You could use the small angle cleavage technique. It is relatively inexpensive and easy to learn. It also works well with glass.
You can use the standard cross sectional method of Bravman and Sinclair. You can take two pieces of your glass slides about 5-10 mm x 10-20 mm and epoxy them together. I use Epo-Tek 353ND, but you can also use N-bond 610. I prefer to use a stack of silicon on one side for a number of reasons: 1) I believe that the Si helps reduce the charging effects, 2) I believe that the Si helps prevent the glass from heating under the beam, 3) I can use the Si to gauge the thickness of the sample during dimple grinding, and 4) the Si can help me find the orientation of the sample relative to the beam that puts the surface parallel to the beam. Cut the samples with a thickness of about 400-500 um with a diamond wheel cutoff saw, hand lap them with a hand grinding tool with parallel sides to between 60-90 um thick, dimple grind them to about 5 um (the Si will show a rich red color in transmitted light), and ion mill to perforation and electron transparency.
You can use Tripod polishing with a low angle ion mill clean-up. This takes some learning to do properly and specialized tools.
You can use an FIB. Glass cuts reasonable well without too much charging affects. Protect the surface with a relatively thick sputter coat of gold or Au-Pd before you put it in the FIB, especially if you use a single beam FIB.
With your finished sample, I found that at 125 kV I had to put a light carbon coat on the sample to prevent softening of the glass under the beam. AT higher voltages (200 kV or better), you don't need to coat the sample for charging or for eliminating the heating effects.
-Scott
Scott D. Walck, Ph.D. PPG Industries, Inc. Glass Technology Center Guys Run Rd. (packages) P. O. Box 11472 (letters) Pittsburgh, PA 15238-0472
Walck-at-PPG.com
(412) 820-8651 (office) (412) 820-8161 (fax)
-----Original Message----- From: Tracy Anderson [mailto:tanderson-at-surmodics.com] Sent: Thursday, January 04, 2001 4:29 PM To: 'Microscopy ListServer' Subject: TEM sample prep for glass slide
--------------------------------------------------------------- --------- 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
Greetings. I would like to look at a cross section of a standard sized glass slide under TEM. Does anyone know how I could prepare such a sample? Will a microtome work? Any suggestions would be very much appreciated.
Tracy E. Anderson Surface Characterization Specialist SurModics, Inc. 952.829.2720 Voice 952.829.2743 Fax tanderson-at-surmodics.com
} This equipment specially designed to work with "image plates". Nothing } related to the negatives. Moreover, they claimed that their system is } supposed to substitute the regular photo-process (and in some instances } that works better, linearity and sensitivity, for instance). Only one } disadvantage - very pricey and time consuming.
Yes, they are better for diffraction work (high dynamic range, linearity). But why time consuming? You just put the plates in the scanner and go do some other things. When you are back you have all the images scanned. No development and stuff like with films.
Best regards,
Rado
--------------------------------------------------------------------- Radostin Danev Laboratory of Ultrastructure Research National Institute for Physiological Sciences Myodaiji-cho, Okazaki 444-8585, JAPAN e-mail: rado-at-nips.ac.jp ---------------------------------------------------------------------
} I am using regular EPSON Expression 1600 flatbed scanner with "transparency } adapter". It has 1600 optical dpi resolution and pretty fast.
Have you tested the MTF of the EPSON? I'm interested what are the actual resolutions X,Y.
Best regards,
Rado
--------------------------------------------------------------------- Radostin Danev Laboratory of Ultrastructure Research National Institute for Physiological Sciences Myodaiji-cho, Okazaki 444-8585, JAPAN e-mail: rado-at-nips.ac.jp ---------------------------------------------------------------------
We have a Tektronix Phaser 780 color laser-printer which is currently out of service. We can not find anyone in Oklahoma who can service it; Xerox, who purchased the Tektronix printer line, is not providing service for this printer.
I wonder if any of you who have this printer have a service source? We seek a service center in the Oklahoma-Texas-Kansas-Arkansas-Misouri area, but are nearly desperate enough to ship this thing anywhere in the U.S.
Thanks, in advance, for any help you provide.
Winton Cornell
--
Winton C. Cornell, Ph.D. Department of Geosciences College of Engineering and Natural Sciences The University of Tulsa Tulsa, OK 74104 phone: 918-631-3248 fax: 918-631-2091 e-mail: winton-cornell-at-utulsa.edu
Sorry I do not know the sizes of the scintillators in the 4500/4700 SEM but the only change you should see is that you run the "contrast" at a lower level than you did prior to the change.
Work we have carried out suggests an improvement compared with the conventional product. Scintilltors start when new with a high signal that falls off quite quickly to start with then there is a gradual decline over the life of the scintillator. In my mind people do not change, or in your future case clean, the scintilltors enough.
Good luck
Steve Chapman Senior Consultant Protrain For consultancy and training by professionals World Wide Tel +44 1280 814774 Fax +44 1280 814007 www.emcourses.com
In an episode of the "X-Files" the EM operator looks up from the TEM and shows Scully the alien virus. It turns out to be an SEM of a pollen grain.
After telling the story to visitors I remind them that any scientist who reveals important information to either Mulder or Scully must take great care when driving home!
Dave
On Wed, 03 Jan 2001 14:25:03 -0600 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 } -----------------------------------------------------------------------. } } } Anyone else happen to watch "Mysterious Ways" earlier this week. One } character was chatting with another about the fantastic new TEM they were } using with the "Kevex EDS system with the twin Quantum 10-mm2 detectors". I } had to listen quick to hear it. } } Granted, its a bit dated (Thermo-Noran is now the name and they don't list } the Quantum on their web page), and some of their other references to other } techniques were of questionable accuracy. Still, I was tickled to see a } reference to EM on TV. I remember a few references on "Quincy", but not a } lot since. } } Disclaimer - I don't have a twin Quantum system, but am still using a } 10-mm2 Quantum on our JEOL-840. } } Warren S. } }
---------------------------------------- Patton, David Email: David.Patton-at-uwe.ac.uk "University of the West of England"
Perhaps you could get a lab with no problems to make some knives with your glass and then test them in their lab and yours (get them to send some of their glass to you as well to test your knifemaker). That should show if it is the glass, the knifemaker or the ultramicrotome that is at fault.
Dave
On Wed, 3 Jan 2001 08:04:10 -0800 "Brownell, Patrick" {patrick.brownell-at-weyerhaeuser.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 } -----------------------------------------------------------------------. } } } My problem is a poor knife edge. The knife looks fine under casual } observation, or with small magnification, but when it comes time to actually } do some sectioning, I get a lot of chattering, or streaking, or both. I } know make as many test blocks as I do sample blocks, so I don't waste } samples with all the bad glass knifes. I've gone through several boxes of } glass over the past two months, and only get a useable knife every 15 to 20 } breaks. The same knife breaker has worked fine in the past, and I have } changed the scoring wheel, and checked all that I can. } } This knife breaker is also very hard to get parts for. The only obvious } problem is that one of the pressure points has a rubber pad that is unevenly } worn. I don't see how that would cause my problem. Again, the knifes look } good to the naked eye. } } The glass I use is from Electron Microscopy Sciences. They are called ultra } glass knife strips 6.5mm x 25mm x 400 mm. } } I guess I'm just looking for someone who has had a similar problem, and } fixed it in some manner. Could I have gotten a bad batch of glass? I don't } think it is very likely, I've used several boxes, but they may all be from } the same batch, for all I know. Is there another brand of glass, or breaker } that others have found produce reliable knives? } } Thanks for any and all help } } -Patrick Brownell } } ---------- } } From: Katja M. Wolski[SMTP:kwolski-at-hsc.usf.edu] } } Reply To: kwolski-at-hsc.usf.edu } } Sent: Wednesday, January 03, 2001 4:26 AM } } To: Brownell, Patrick } } Subject: Re: Ralph Glass Knife problems } } } } I use a different knife machine, but what's the problem you're having? } } Are you } } not getting a good knife edge or what? } } } } Katja } } } } } } } } "Brownell, Patrick" 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 use Ralph type glass knives for plastic sectioning of biological } } samples. } } } I am experiencing problems in making a proper knife. I have a TAAB } } } histoknifemaker (also says Reichart-Jung). Is there anyone willing to } } offer } } } expertise in this area? } } } } } } -Patrick Brownell } } }
---------------------------------------- Patton, David Email: David.Patton-at-uwe.ac.uk "University of the West of England"
I don't know the machine, but is TAAB no longer in business in the UK? For the longest time TAAB supplies (altho not generally easily available in the US) was an excellent source of resins and small items. Regardless, I would think that the worn rubber pad is your problem. Again, thinking of experience with other knifemakers, the pads are an essential part of relieving some of the stress in the glass as it breaks. If this pad is uneven, it may not be absorbing the pressure/stress as it should. Perhaps (if TAAB is not around) some other users of the knifemaker might have accessories (like a spare pad) to help you out. Also check the following: depth of the score--if it's too deep or too light, that will affect the break and edge quality; how fast are you breaking after scoring? - a slow break has always been essential to consistently good knife edges for me; check the setting of the clamp(s) and pressure points to ensure that there are no uneven points and that the clamp(s) are providing equal pressure. I can't find the reference right now, but the original publications on making the Ralph knives by hand (it was in Stain Technology, I think) might get you by, and it also might allow you to check the quality of the glass. The technique wasn't too difficult or tedious, and, as I remember (from the dim recesses of ancient history) the percentage of good knives was acceptable. Hope this helps.
Roger Moretz, Ph.D. Dept of Toxicology Boehringer Ingelheim Pharmaceuticals, Inc.
On Fri, 5 Jan 2001 09:21:24 +0000 (GMT Standard Time), Patton, David 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 } -----------------------------------------------------------------------. } } } Perhaps you could get a lab with no problems to make some } knives with your glass and then test them in their lab and } yours (get them to send some of their glass to you as } well to test your knifemaker). That should show if it is } the glass, the knifemaker or the ultramicrotome that is at } fault. } } Dave } } } On Wed, 3 Jan 2001 08:04:10 -0800 "Brownell, Patrick" } {patrick.brownell-at-weyerhaeuser.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 } } -----------------------------------------------------------------------. } } } } } } My problem is a poor knife edge. The knife looks fine under casual } } observation, or with small magnification, but when it comes time to actually } } do some sectioning, I get a lot of chattering, or streaking, or both. I } } know make as many test blocks as I do sample blocks, so I don't waste } } samples with all the bad glass knifes. I've gone through several boxes of } } glass over the past two months, and only get a useable knife every 15 to 20 } } breaks. The same knife breaker has worked fine in the past, and I have } } changed the scoring wheel, and checked all that I can. } } } } This knife breaker is also very hard to get parts for. The only obvious } } problem is that one of the pressure points has a rubber pad that is unevenly } } worn. I don't see how that would cause my problem. Again, the knifes look } } good to the naked eye. } } } } The glass I use is from Electron Microscopy Sciences. They are called ultra } } glass knife strips 6.5mm x 25mm x 400 mm. } } } } I guess I'm just looking for someone who has had a similar problem, and } } fixed it in some manner. Could I have gotten a bad batch of glass? I don't } } think it is very likely, I've used several boxes, but they may all be from } } the same batch, for all I know. Is there another brand of glass, or breaker } } that others have found produce reliable knives? } } } } Thanks for any and all help } } } } -Patrick Brownell } } } ---------- } } } From: Katja M. Wolski[SMTP:kwolski-at-hsc.usf.edu] } } } Reply To: kwolski-at-hsc.usf.edu } } } Sent: Wednesday, January 03, 2001 4:26 AM } } } To: Brownell, Patrick } } } Subject: Re: Ralph Glass Knife problems } } } } } } I use a different knife machine, but what's the problem you're having? } } } Are you } } } not getting a good knife edge or what? } } } } } } Katja } } } } } } } } } } } } "Brownell, Patrick" 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 use Ralph type glass knives for plastic sectioning of biological } } } samples. } } } } I am experiencing problems in making a proper knife. I have a TAAB } } } } histoknifemaker (also says Reichart-Jung). Is there anyone willing to } } } offer } } } } expertise in this area? } } } } } } } } -Patrick Brownell } } } } } } } ---------------------------------------- } Patton, David } Email: David.Patton-at-uwe.ac.uk } "University of the West of England" } }
_______________________________________________________ Send a cool gift with your E-Card http://www.bluemountain.com/giftcenter/
On Fri, 5 Jan 2001 05:28:34 -0800 (PST) Roger Moretz {rcmoretz-at-excite.com} wrote:
} Patrick: } } I don't know the machine, but is TAAB no longer in business in the UK? For } the longest time TAAB supplies (altho not generally easily available in the } US) was an excellent source of resins and small items. Regardless, I would } think that the worn rubber pad is your problem. Again, thinking of } experience with other knifemakers, the pads are an essential part of } relieving some of the stress in the glass as it breaks. If this pad is } uneven, it may not be absorbing the pressure/stress as it should. Perhaps } (if TAAB is not around) some other users of the knifemaker might have } accessories (like a spare pad) to help you out. Also check the following: } depth of the score--if it's too deep or too light, that will affect the } break and edge quality; how fast are you breaking after scoring? - a slow } break has always been essential to consistently good knife edges for me; } check the setting of the clamp(s) and pressure points to ensure that there } are no uneven points and that the clamp(s) are providing equal pressure. I } can't find the reference right now, but the original publications on making } the Ralph knives by hand (it was in Stain Technology, I think) might get you } by, and it also might allow you to check the quality of the glass. The } technique wasn't too difficult or tedious, and, as I remember (from the dim } recesses of ancient history) the percentage of good knives was acceptable. } Hope this helps. } } Roger Moretz, Ph.D. } Dept of Toxicology } Boehringer Ingelheim Pharmaceuticals, Inc. } } On Fri, 5 Jan 2001 09:21:24 +0000 (GMT Standard Time), Patton, David 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 } } -----------------------------------------------------------------------. } } } } } } Perhaps you could get a lab with no problems to make some } } knives with your glass and then test them in their lab and } } yours (get them to send some of their glass to you as } } well to test your knifemaker). That should show if it is } } the glass, the knifemaker or the ultramicrotome that is at } } fault. } } } } Dave } } } } } } On Wed, 3 Jan 2001 08:04:10 -0800 "Brownell, Patrick" } } {patrick.brownell-at-weyerhaeuser.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 } } } } -----------------------------------------------------------------------. } } } } } } } } } My problem is a poor knife edge. The knife looks fine under casual } } } observation, or with small magnification, but when it comes time to } actually } } } do some sectioning, I get a lot of chattering, or streaking, or both. } I } } } know make as many test blocks as I do sample blocks, so I don't waste } } } samples with all the bad glass knifes. I've gone through several boxes } of } } } glass over the past two months, and only get a useable knife every 15 } to 20 } } } breaks. The same knife breaker has worked fine in the past, and I have } } } changed the scoring wheel, and checked all that I can. } } } } } } This knife breaker is also very hard to get parts for. The only } obvious } } } problem is that one of the pressure points has a rubber pad that is } unevenly } } } worn. I don't see how that would cause my problem. Again, the knifes } look } } } good to the naked eye. } } } } } } The glass I use is from Electron Microscopy Sciences. They are called } ultra } } } glass knife strips 6.5mm x 25mm x 400 mm. } } } } } } I guess I'm just looking for someone who has had a similar problem, and } } } fixed it in some manner. Could I have gotten a bad batch of glass? I } don't } } } think it is very likely, I've used several boxes, but they may all be } from } } } the same batch, for all I know. Is there another brand of glass, or } breaker } } } that others have found produce reliable knives? } } } } } } Thanks for any and all help } } } } } } -Patrick Brownell } } } } ---------- } } } } From: Katja M. Wolski[SMTP:kwolski-at-hsc.usf.edu] } } } } Reply To: kwolski-at-hsc.usf.edu } } } } Sent: Wednesday, January 03, 2001 4:26 AM } } } } To: Brownell, Patrick } } } } Subject: Re: Ralph Glass Knife problems } } } } } } } } I use a different knife machine, but what's the problem you're } having? } } } } Are you } } } } not getting a good knife edge or what? } } } } } } } } Katja } } } } } } } } } } } } } } } } "Brownell, Patrick" 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 use Ralph type glass knives for plastic sectioning of biological } } } } samples. } } } } } I am experiencing problems in making a proper knife. I have a TAAB } } } } } histoknifemaker (also says Reichart-Jung). Is there anyone willing } to } } } } offer } } } } } expertise in this area? } } } } } } } } } } -Patrick Brownell } } } } } } } } } } } ---------------------------------------- } } Patton, David } } Email: David.Patton-at-uwe.ac.uk } } "University of the West of England" } } } } } } } } } } _______________________________________________________ } Send a cool gift with your E-Card } http://www.bluemountain.com/giftcenter/ } }
---------------------------------------- Patton, David Email: David.Patton-at-uwe.ac.uk "University of the West of England"
Are you vacuum embedding the glass and Spurr's resin? That should work to get a lot of the void space out.
Just pour the resin into the embedding capsule, put the capsule into a vacuum oven, let pump down for a few minutes (~20 min), bring the sample back to room pressure to let the air pressure force the resin into the pores, then pump it down again and bring back to room pressure and let the sample cure.
dz
David Ziegler U.S. Army, SBCCOM AMSSB-RSS-MS(N) Materials Science Team, SS&T Natick, MA 01760-5020 TEL: (508) 233-6484 FAX: (508) 233-5521 Email: David.Ziegler-at-Natick.Army.Mil
} As part of the planned makeover of our building, it has been } proposed ... } Part of that proposal was to set up a computing lab with } fileserver and work-stations networked ... } However, there is great pressure on space in this building, and it } has been suggested to me that computing for imaging and } spectroscopy does not need to be separated from general purpose } computing these days. ...
Somewhat true ... for our EPMA and SEM images, we simply archive to a "files available" location, and every researcher has their own computer and software. However, you would need a workstation for the OM, would you not?
Can anyone answer this question . Remember Ask-A-Microscopist is a forum that is used by NON-MICROSCOPISTS looking for help so keep try to your technical details at the right level.
Email: us004118-at-mindspring.com Name: Leonard Lessin, FBPA
School: (Retired Science & Medical Photographer)
State: NY
Zip: 10012
Question: I am enjoying doing photomicrographs of crystal preperations in polarized light.However I have insuffient knowledge of chemistry to choose solvents without a long series of trial and error efforts.Can you give me a rationale and/or a reference to go about this in a more productive manner?
High quality professional film scanners (LeafScan 45, LS-4500 etc.) are very expansive - over $10k.
I use MINOLTA Dimage Scan Multi (Minolta USA -- how2scan.com ) for digitizing of TEM negatives.
Its features: - Optical resolution: 1128dpi (TEM) 2820dpi (35mm, APS) - Dynamic range: 3.6 - Price: around $2,000
It has one drawback only: TEM film adapter aperture size is of 2.2x3.15. However only central part of a negative is used for image processing.
There is a choice among the price and convenience.
Best regards,
Alexander
Dr. A.S. Solodukhin Department of Anesthesiology University of Virginia Health System P.O. Box 800710 Charlottesville, VA 22906-0710 FAX : (804) 982-0019 Phone: (804) 924-2494
"Dr. Catherine Powell" 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 a clinical diagnostic TEM laboratory serving a provincial network of hospitals. We would like to move away from conventional darkroom printing of images and wish to convert negatives to digital files. We are looking for a negative scanner that will: } } 1. Accept 3 X 4 1/4 inch sheet film negatives (Kodak 4489 film). } } 2. Comes with software support that is adaptable to a Windows format. } } 3. Must be priced under $3000. } } 4. Must provide the best quality resolution for diagnostic results (i.e. 3200 X 3600 pixel; wide linear dynamic range). } } I look forward to any information and advice you can provide. } } Catherine Powell } }
Since there has been only one other response, I will toss in my 2 cents.
Some time back I would have said that the load of microscopic images would be more than what the general purpose computing lab would want to take responsibility for. It might prove a significant network traffic load too. However, I think any decent network should be able to handle the load from the microscope labs. On the side, we have a good campus network here at Iowa State. However an analysis of network traffic shows a disproportionate amount of traffic coming out of a few dorm rooms (the normal traffic pattern would be incoming). The university is going to start limiting traffic to so many gigabytes per month or start charging. So I think the microscope load is no longer that significant.
The other issue that might work against it is software licensing. I don't know if you use special programs to work with your images. It might be difficult to work out a suitable licensing arrangement if that software needs to be installed on a lab full of computers, but maybe you can.
As far as regular maintenance of the data, I would be all in favor of letting someone else do the backups providing they have the space (and they should).
Warren
At 06:25 PM 1/2/2001 +0000, you wrote:
} As part of the planned makeover of our building, it has been } proposed that the various and somewhat distributed microscopy } facilities in our building - SEM, TEM, Confocal, fluorescence, } luminescence imaging, darkroom etc. etc. might be brought together } to form a biological imaging facility, thereby benefitting from some } improvements in supervision, security and user support. Part of that } proposal was to set up a computing lab with fileserver and work- } stations networked to the instruments and dedicated to image } storage and off-line image and spectral processing and analysis. } However, there is great pressure on space in this building, and it } has been suggested to me that computing for imaging and } spectroscopy does not need to be separated from general purpose } computing these days. What are your opinions about this? Pro or } con? } } Happy New Millennium } Chris } ~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~ } Dr Chris Jeffree } University of Edinburgh
---------------------- Warren E. Straszheim Materials Analysis and Research Lab Iowa State University 23 Town Engineering Ames IA, 50011-3232
we're looking to buy a used carbon evaporator and before I speed through the used equipment websites I thought I'd just check to see if anyone here is thinking of selling their one.
cheers Liz McKenzie
******************************************************* Geomicrobiology and Electron Microscopy Laboratory Room S9 Cramer Hall 1721 SW Broadway Portland State University Portland OR97201
Applications of Scanning Microscopy in Forensic Science
Dear Fellow Microscopist / Forensic Scientist,
SCANNING 2001, the Thirteenth Annual International Scientific Meeting on Scanning Microscopies will be held May 5-7, 2001, in New York City at The Roosevelt Hotel. Please make plans to attend three full days of scientific papers and six short courses all devoted to the use of scanning microscopy. Numerous specific application topics including forensics, electron backscattered diffraction, scanning probe microscopy, nanotechnology, anthropology, modern optical microscopy, museum applications of SEM, food microstructure, material science, microwave techniques and pharmaceuticals. For a completely listing of session topics, short course titles and registration information, please visit the SCANNING web site at www.scanning-fams.org.
CALL FOR PAPERS:
As a co-chair of the SCANNING 2001's "Applications of Scanning Microscopy in Forensic Science" session, I am most pleased with the participation and interest in the forensic session over the last eight years. This year, Mr. Dennis Ward of the Federal Bureau of Investigation, has graciously agreed to co-chair the forensic sessions. Together, we are planning to provide an exciting and informative forensic program. The continued growth of the forensic session over the last eight years will once again permit two full days of forensic papers. The "Applications of Scanning Microscopy in Forensic Science" sessions will be held on Sunday and Monday, May 6-7, 2001. Combined with the popular one day "Scanning Microscopy in Forensic Science" short course (Saturday, May 5, 2001), the forensic scientist/student will be able to attend three consecutive (and full) days of instruction as well as scientific papers on current forensic science research and unique cases all devoted to scanning microscopy applications in forensic science. A large number of microscopy vendors and a full schedule of social activities and tours in New York are also available for a most enjoyable meeting experience.
I encourage you to submit an abstract for platform or poster consideration and be a part of the SCANNING 2001 Forensics Session. Additionally, if you are involved with or know of forensic science students actively engaged in forensic research using any type of scanning microscopy, I strongly encourage you to have your student(s) submit an abstract for consideration as a student paper or poster. Again, please visit the SCANNING web site at www.scanning-fams.org.
Should you have any questions about the forensic symposium, short course or student papers, please feel free to contact me.
See you in New York!
S. Frank Platek, MS Co-Chair, Forensic Symposium and Short Course SCANNING 2001 (513) 679-2700 (513) 679-2761 FAX fplatek-at-ora.fda.gov
Looking for a few good Account Representatives for an electron and optical microscopy service. Territory is open. Excellent earning potential. Call Dick O'Connell at 734-668-3309 or e-mail at oconnell-at-ltu.edu for more information.
I believe TAAB is still in business TAAB Laboratories Equipment Ltd. 3 Minerva House Calleva Park Aldermaston , Berkshire RG7 8NA UK Phone: 44-118-9817775 Fax: 44-118-9817881 E-mail: sales-at-taab.co.uk
Chris
----- Original Message ----- } From: "Roger Moretz" {rcmoretz-at-excite.com} To: "Patton, David" {David.Patton-at-uwe.ac.uk} ; "Brownell, Patrick" {patrick.brownell-at-weyerhaeuser.com} Cc: "'Microscopy-at-MSA.Microscopy.Com'" {Microscopy-at-sparc5.microscopy.com} Sent: Friday, January 05, 2001 1:28 PM
The earliest mention of EM in TV or movies goes back in time much further than "Quincy" or the "X-Files".
I thought I would mention my favorite EM TV/Movie memory. Anyone remember the movie called "The Andromeda Strain" ?? The movie from the 60's was based on a Michael Crighton book by the same name . A Transmission Electron Microscope (RCA EMU ???), as well as "live" images of the ultramicrotomy sectioning process were featured.
Remember?
I would be interested in knowing if there are earlier references than this one.
Best Wishes,
Bill Monroe -- Bill Monroe EM Center Mississippi State University (601)-325-3019 Lab Fax 325-0246
You're correct about the RCA microscope, except that the one in the movie was right after RCA discontinued the business, and it was picked up by "Forgflo", which was the name seen clearly in the movie.
Check it out...
Larry (Master of all trivia...why don't I get on Who Wants to be a Millionaire?) ;-)
} ------------------------------------------------------------------------ } 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 earliest mention of EM in TV or movies goes back in time much } further than "Quincy" or the "X-Files". } } I thought I would mention my favorite EM TV/Movie memory. Anyone } remember the movie called "The Andromeda Strain" ?? The movie from } the 60's was based on a Michael Crighton book by the same name . A } Transmission Electron Microscope (RCA EMU ???), as well as "live" } images of the ultramicrotomy sectioning process were featured. } } Remember? } } I would be interested in knowing if there are earlier references } than this one. } } Best Wishes, } } Bill Monroe } -- } Bill Monroe } EM Center } Mississippi State University } (601)-325-3019 Lab } Fax 325-0246
Dr. Lawrence F. Allard Senior Research Staff Member High Temperature Materials Laboratory Oak Ridge National Laboratory 1 Bethel Valley Road Bldg. 4515, MS 6064 PO Box 2008 Oak Ridge, TN 37831-6064
You might also recall that in the Andromeda Strain movie, the specimen was inserted through the viewing port and placed on the fluorescent screen. In this way the were actually able to watch the "virus" replicate right before their eyes.
At 02:39 PM 01/05/2001 -0600, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Gregory W. Erdos, Ph.D. Assistant Director, Biotechnology Program PO Box 110580 University of Florida Gainesville, FL 32611
----- Original Message ----- } From: "Warren E Straszheim" {wesaia-at-iastate.edu} {snip}
} } As far as regular maintenance of the data, I would be all in favor of } letting someone else do the backups providing they have the space (and they } should).
Warren,
If the backups are of any value to you the only person you can trust to make them is yourself. The only method I have found that has never failed me it to compress the files in zip format transfer it to the backup media and verify it on the back up media. Then store the back up media off site. The zip format applies to MSDOS computer other archive file types apply to other OSs.
If the data is really important make two copies.
Unless you can hire a lot better folks then I have seen colleges hire they will make mistakes on backups sooner or later probably sooner.
Gordon Gordon Couger gcouger-at-couger.com Stillwater, OK www.couger.com/gcouger 405 624-2855 GMT -6:00
Of course some of us remember this movie but for heavens sake why did they have green "colored" (interference "color") sections floating in the microtome knife boat when gold surely would have photographed as well and fit the dialogue of that scene. Obviously the technical people just said well cut us some sections to phtograph. A sore point to me at the time.
} } } "William A. Monroe" {monroe-at-emcenter.msstate.edu} 01/05 12:39 PM } } } ------------------------------------------------------------------------ The Microscopy ListServer -- Sponsor: The Microscopy Society of America
The earliest mention of EM in TV or movies goes back in time much further than "Quincy" or the "X-Files".
I thought I would mention my favorite EM TV/Movie memory. Anyone remember the movie called "The Andromeda Strain" ?? The movie from the 60's was based on a Michael Crighton book by the same name . A Transmission Electron Microscope (RCA EMU ???), as well as "live" images of the ultramicrotomy sectioning process were featured.
Remember?
I would be interested in knowing if there are earlier references than this one.
Best Wishes,
Bill Monroe -- Bill Monroe EM Center Mississippi State University (601)-325-3019 Lab Fax 325-0246
The other fun thing about the crystalline image in that TEM from Andromeda Strain was that it was in color!
-Scott
Scott D. Walck, Ph.D. PPG Industries, Inc. Glass Technology Center Guys Run Rd. (packages) P. O. Box 11472 (letters) Pittsburgh, PA 15238-0472
Walck-at-PPG.com
(412) 820-8651 (office) (412) 820-8161 (fax)
-----Original Message----- From: William A. Monroe [mailto:monroe-at-emcenter.msstate.edu] Sent: Friday, January 05, 2001 3:39 PM To: Warren E Straszheim Cc: Microscopy-at-sparc5.microscopy.com Subject: Re: TV Trivia
--------------------------------------------------------------- --------- 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/MicroscopyListserv er/FAQ.html
The earliest mention of EM in TV or movies goes back in time much further than "Quincy" or the "X-Files".
I thought I would mention my favorite EM TV/Movie memory. Anyone remember the movie called "The Andromeda Strain" ?? The movie from the 60's was based on a Michael Crighton book by the same name . A Transmission Electron Microscope (RCA EMU ???), as well as "live" images of the ultramicrotomy sectioning process were featured.
Remember?
I would be interested in knowing if there are earlier references than this one.
Best Wishes,
Bill Monroe -- Bill Monroe EM Center Mississippi State University (601)-325-3019 Lab Fax 325-0246
"Scanned Probe and Electron Microscopy and Microanalysis: Applications & Techniques" _________________________________________________________________________
The University of Sydney
February 14-16, 2001
AMAS and ASPMS invite you to join us for what will probably be the very first electron and scanned probe microscopy meeting of the 21st Century.
The aim of the Symposium is to provide a forum where participants can discuss electron and scanned probe microscopy, with emphasis on practical solutions and applications. A number of overseas invited speakers will be involved with both the Symposium and the Workshops. We also encourage you to present your recent work using SPM, SEM/TEM and microanalysis.
Pre-Symposium Workshop February 12-13, 2001 Practical Digital Imaging Introduction to SPM Spectral Imaging Materials SPM Environmental SEM Biological SPM Low Voltage SEM and microanalysis SPM of Soft Materials Advances in EBSD in SEM SPM Calibration and Maintenance Introduction to XEDS and EELS in the EM Functionalising Tips
Information concerning the symposium, workshops, accommodation, registration, etc. is posted on our website (www.microscopy.org.au then follow the link to "Upcoming ASPMS, AMAS Symposium". This information will be revised and expanded as necessary.
Just a word of caution about Zip disks. They can be very unreliable. When Iomega first came out with them, their media was really good. Now it is not the same. Maxell and Fujifilm also make media. I think that theirs are better.
The other problem with Iomega drives (Zip and Jaz) is the click of death. This is a precursor to a dead drive or media and loss of all that is on the media (if bad media).
To check your drives and media, run tip.exe. To find out more about this, visit http://www.grc.com
gary g.
At 01:53 PM 1/5/01, you wrote:
} ----- Original Message ----- } } From: "Warren E Straszheim" {wesaia-at-iastate.edu} } {snip} } } } } } As far as regular maintenance of the data, I would be all in favor of } } letting someone else do the backups providing they have the space (and } they } } should). } } Warren, } } If the backups are of any value to you the only person you can trust to } make them is yourself. The only method I have found that has never failed } me it to compress the files in zip format transfer it to the backup media } and verify it on the back up media. Then store the back up media off site. } The zip format applies to MSDOS computer other archive file types apply to } other OSs. } } If the data is really important make two copies. } } Unless you can hire a lot better folks then I have seen colleges hire they } will make mistakes on backups sooner or later probably sooner. } } Gordon } Gordon Couger gcouger-at-couger.com } Stillwater, OK www.couger.com/gcouger } 405 624-2855 GMT -6:00
Yes....different "zip." Winzip is very good for munching files into a smaller data space. The media problem remains, however. As you point out, other media keeps coming out.
I tried DVD-RAM and really got whacked by bad sectors. I don't use that any longer. DVD-R is quite another story. CD-R is so cheap these days it is a great way to store 600MB of data. The only problem is to ensure that it remains on the media. Most burner programs do not verify after write. Toast on the Mac does, but Adaptec's programs on the PC do not. I have not found any other programs that will verify after write on the PC. Bummer.
I have not done much at all with CD-RW. I wonder what the experiences have been with this option? My new Yamaha drive is 16x/10x/40x and should do nicely for RW. Never tried it for RW. I guess that I should do that some day. CD-Rs at 12X are iffy....even with certified media. That's why the verification is such an important missing feature.
For really good backup and restore, consider the removable IDE drives. Very nice. My one year's work fits on three 45G drives. Hopefully it remains accessible in the future. Data overload is an emerging problem.
gg
At 08:03 PM 1/5/01, you wrote:
} ----- Original Message ----- } From: "Gary Gaugler" {gary-at-gaugler.com} } To: "Gordon Couger" {gcouger-at-couger.com} } Cc: "MSA listserver" {Microscopy-at-sparc5.microscopy.com} } Sent: Friday, January 05, 2001 7:16 PM } Subject: Re: Computing for microscopy and imaging } } } } Just a word of caution about Zip disks. They can be very } } unreliable. When Iomega first came out with them, their } } media was really good. Now it is not the same. Maxell } } and Fujifilm also make media. I think that theirs are better. } } } } The other problem with Iomega drives (Zip and Jaz) is the } } click of death. This is a precursor to a dead drive or } } media and loss of all that is on the media (if bad media). } } } } To check your drives and media, run tip.exe. To find out } } more about this, visit http://www.grc.com } } } } gary g. } } Gary, } } Zip files not Zip disk. Use Pkzip or some other program to put all the } files into one zip file, usually a complete directory, copy that file to } the back up media and verify the zip file on the back up media. Currently } I use write only CD-ROMs and keep a copy of really important stuff on my } internet server at my ISP as well. Hard disk space is cheap. I have the } last 15 years work at my finger tips. If I can find it:) I started using } this on single sided single density floppies on a Radio Shack Model 1. I } can only think of two times that I was unable to retrieve a file in 20 } years. } } I am a programmer not a photographer so a years work might fit on a floppy } disk. } } I am not satisfied with the life of CD-ROMs but so far something better } has always come along before the old media went bad and I copied it all } over. One thing I don't like about CD-ROMs is they are not protected from } scratching or being broken. } } Gordon } Gordon Couger gcouger-at-couger.com } Stillwater, OK www.couger.com/gcouger } 405 624-2855 GMT -6:00
----- Original Message ----- } From: "Gary Gaugler" {gary-at-gaugler.com} To: "Gordon Couger" {gcouger-at-couger.com} Cc: "MSA listserver" {Microscopy-at-sparc5.microscopy.com} Sent: Friday, January 05, 2001 10:59 PM
I am looking for accessories and parts for binocular microscope Jenna Technoval 2. Anyone have some spare unneeded accessories as camera attachment, oculars, literature, etc?
Keep care and be of good cheer.
Regards
(name) Vratislav Richard Eugene Maria John Baptist (surname) of Bejsak (Bayshark)-Colloredo-Mansfeld
website: http://www.coleoptera.org listserver: coleoptera on www.egroup.com/group/coleoptera/info.html Coleoptera - Australia, Tenebrionidae of World (incl. Lagriinae, Alleculinae)
University of Sydney The Wentworth Bldg., Box 62 NSW 2006 AUSTRALIA phone : +61 414 540 465 email: vratislav-at-bigfoot.com ricardo-at-ans.com.au (before Ricardo-at-compuserve.com and ricardo-at-login.cz )
Only after the last tree has been cut down, only after the last river has been poisoned, only after the last fish has been caught, only then will you find that money can not be eaten.' CREE INDIAN PROPHECY.
Incoming mail is certified Virus Free. Checked by AVG anti-virus system (http://www.grisoft.com).
In one of the Batman movies where he fights the arch villain Mr. Freeze. In the part of the move where the police raid Mr. Freezes' lair you will see off to one side a Philips 400 TEM dressed up as a cheap prop. This is an insult to the Scientist and Technicians who have developed finely honed skills to bring to light the world of the very small in a effort to make life a little better for all of us. Electron Microscopy has been an important part of Science for the last half of the 20th century. This finely engineered tool of Science has open up the world of the very small to eyes that would never have imagined that life could exist on such a level. It sickens me to see this fine and noble tool of Science reduced to a carnival side show gimmick. It is my hope that the men and women of this newsgroup will in their own way and in their own time bring electron microscopy back to its proper place in the scientific community, because if we of this newsgroup and others who labor in Science do not, than this important source of knowledge will be lost to history and the politicians. I will now get off my soap box and make no further comment on the subject.
Ronald Austin Research Associate LSU Medical Center Dept of Pathology Shreveport, LA rla-at-mindspring.com
-----Original Message----- } From: Rosemary White [mailto:Rosemary.White-at-pi.csiro.au] Sent: Friday, January 05, 2001 11:52 PM To: Microscopy-at-sparc5.microscopy.com
And there were all those Zeiss microscopes in Jurassic Park. Pity the one they were using in one scene (an Axiophot?) didn't have a condenser....
Rosemary White Microscopy Centre CSIRO Plant Industry GPO Box 1600 Canberra, ACT 2601 Australia
Ah, come on. There were many technical errors in that film, but wasn't it fun? One of my favorite faux pas was the rapid growth? multiplication? of the strain. Not to mention it's apparent ability to degrade a variety of natural and synthetic rubbers while also attacking human blood plasma.
Michael Crichton did a good job of describing a possible protagonist, and Hollyweird did its usual job of visualizing it. To expect anything different would be folly.
On Friday, January 05, 2001 4:59 PM, Walck, Scott D. [SMTP:walck-at-ppg.com] wrote: } } The other fun thing about the crystalline image in that TEM from Andromeda Strain was that it was in color! } } } -Scott } } -----Original Message----- } From: William A. Monroe [mailto:monroe-at-emcenter.msstate.edu]
} } The earliest mention of EM in TV or movies goes back in time much } further than "Quincy" or the "X-Files". } } I thought I would mention my favorite EM TV/Movie memory. Anyone } remember the movie called "The Andromeda Strain" ?? The movie from } the 60's was based on a Michael Crighton book by the same name . A } Transmission Electron Microscope (RCA EMU ???), as well as "live" } images of the ultramicrotomy sectioning process were featured. } } Remember? } } I would be interested in knowing if there are earlier } references than this one. } } Best Wishes, } } Bill Monroe } -- } Bill Monroe } EM Center } Mississippi State University } (601)-325-3019 Lab } Fax 325-0246 } } }
Allen R. Sampson, Owner Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174 voice 630.513.7093 fax 630.513.7092
} } Yes....different "zip." Winzip is very good for munching } } files into a smaller data space. The media problem remains, } } however. As you point out, other media keeps coming out. } ============================ } I really think the best media out there for long term storage would be } plain old 35 mm film. I don't know what kind of data density you could get } on tech pan but I would trust the data to be there when I wanted to get it } back.
Winzip does a good job on data that is compressible. Non-LZW TIFF can be compressed as can ASCII and other byte hungry data. But I don't find much size reduction with compressed TIFF or JPEG. These are mostly what I have. Even then, my native images are uncompressed TIFF. Those are what I need to save as backups plus backups of the backups.
} } } } I have not done much at all with CD-RW. I wonder what } } the experiences have been with this option? My new Yamaha } } drive is 16x/10x/40x and should do nicely for RW. Never tried } } it for RW. I guess that I should do that some day. CD-Rs at } } 12X are iffy....even with certified media. That's why the } } verification is such an important missing feature. } =============== } } From the reports I see on RW CDROMs the storage life is a lot shorter than } a R CDROM. Both of them use some kind of dye process and the RW is } reversable.
I too have not heard good things about RW. Unless and until the viability is assured, my precious data isn't going on an RW media. When its gone, its gone. Not a good situation.
} It takes time and markting didn't like it is my guess. But that is why you } have to verify each file you copy with verify option of Winzip. It reads } the file and does the CRC and checks it against the one in the file. } } It is slow and cumbersom but it is the only way I have found that works on } MSDOS or Windos. On Linux or Unix I can write a script to do it all. I } have been involved in disaster recovereries and most of the times at least } part of the back ups are bad. Some of the restore system can't recover } from a bad file. I don't know much about backup systems for contemperary } systems I just copy every thing to a CDROM uncompressed and put a } compressed version on the network box and call it good.
Hum. I'm using Winzip 7 and it is very fast on Win98SE. Stuffit on the Mac also does a nice job.
} } } } For really good backup and restore, consider the removable } } IDE drives. Very nice. My one year's work fits on three 45G } } drives. Hopefully it remains accessible in the future. Data } } overload is an emerging problem. } ================================== } That's what I do on my Linux box on the internet. I have a drive for } backups. Drives are cheap. High quality digital imagining is going to } really eat up disk space. We need 10 or 20 gig CDROMs
Yes indeed. Even a 10G CD would be great, if it worked. I've toyed with the idea of DVD-R which will do 4.7G and 9G. But the drives are very pricey as is the media. And I suspect they may have the same reliability issues as CD-RW and even CD-R. Not all CD-R writes work 100%. Only Toast on the Mac will do a verify after write. I've not found any burner program for the PC that will verify after write. Strange.
The IDE drive trays seem like a good approach to backup. The drives too are obsoleted rather quickly. My "new" IBM 45G Deskstar ATA-66 drives are now discontinued. IBM makes ATA-100 45G drives for $239 versus the $129 I paid for the ATA-66 ones.
My only other backup option (a redundant one) is a Sony SDT-9000 4mm DAT. Using native hardware compression, it will store 24G on a DDS-3 120meter tape. But this has some peculiar problems based on lack of backup software for tape that works in a dual host adapter environment. Dantz's Retrospect works great on the Mac but fails on the PC. I have to use old Win95 Adaptec backup. It works but does not offer user interface to the drive's features.
It seems that as we rush from film to digital, we may look back on the thousands of negs or chromes sitting in file cabinets and wonder what happened. We'd now have file cabinets of $200 hard drives which may or may not work after sitting for some amount of time. A rather unsettling feeling.
Holey Microscopy Batman...maybe we should blame that on Alfred. And to think I didn't tune in the following night...same bat time...same bat channel...to see if this oversight was corrected.
-----Original Message----- } From: Ronald Austin [mailto:rla-at-mindspring.com] Sent: Saturday, January 06, 2001 12:18 AM To: Microscopy Society of America
In one of the Batman movies where he fights the arch villain Mr. Freeze. In the part of the move where the police raid Mr. Freezes' lair you will see off to one side a Philips 400 TEM dressed up as a cheap prop. This is an insult to the Scientist and Technicians who have developed finely honed skills to bring to light the world of the very small in a effort to make life a little better for all of us. Electron Microscopy has been an important part of Science for the last half of the 20th century. This finely engineered tool of Science has open up the world of the very small to eyes that would never have imagined that life could exist on such a level. It sickens me to see this fine and noble tool of Science reduced to a carnival side show gimmick. It is my hope that the men and women of this newsgroup will in their own way and in their own time bring electron microscopy back to its proper place in the scientific community, because if we of this newsgroup and others who labor in Science do not, than this important source of knowledge will be lost to history and the politicians. I will now get off my soap box and make no further comment on the subject.
Ronald Austin Research Associate LSU Medical Center Dept of Pathology Shreveport, LA rla-at-mindspring.com
I have enjoyed reading all the TV trivia regarding the Quincy and Andromeda Strain. What many of you may not know is that for the "Strain" movie the makers of the film contacted a now defunct Microprobe Company, Materials Analysis Co. We sent to the studio an Electron Microprobe. The only portion that made the film was some blinking x-ray scalers and a portion of the electronics rack. What the impact of microprobe was in the film I can't guess or remember. In the Quincy episodes, there were more than one, we sent to the studio an ISI SEM along with a service engineer, whose name at the moment escapes me, to install it and our application and Demonstration man, Bill Roth to run the SEM, Bill has been with Hitachi for many years now and could give more incite as to what happened at the studio than I can as he was there for a week doing the one episode. I remember him telling me that Quincy's technician, Sam was explaining to Quincy what was on the CRT with the camera going from the control panel with Bill's hands being filmed but the overall shot of Sam and Quincy looking at the CRT and discussing the forensic material. I still have some 8x10's around here somewhere of the filming. Thought you might be interested.
{snip} } Winzip does a good job on data that is compressible. Non-LZW TIFF } can be compressed as can ASCII and other byte hungry data. But } I don't find much size reduction with compressed TIFF or JPEG. These } are mostly what I have. Even then, my native images are uncompressed } TIFF. Those are what I need to save as backups plus backups of the } backups. ========= These files are already compressed as much as possible. The only advantage of zip programs they get them in one file. {snip} } } } For really good backup and restore, consider the removable } } } IDE drives. Very nice. My one year's work fits on three 45G } } } drives. Hopefully it remains accessible in the future. Data } } } overload is an emerging problem. } } ================================== } } That's what I do on my Linux box on the internet. I have a drive for } } backups. Drives are cheap. High quality digital imagining is going to } } really eat up disk space. We need 10 or 20 gig CD-ROMs } } Yes indeed. Even a 10G CD would be great, if it worked. I've } toyed with the idea of DVD-R which will do 4.7G and 9G. But } the drives are very pricey as is the media. And I suspect they } may have the same reliability issues as CD-RW and even CD-R. } Not all CD-R writes work 100%. Only Toast on the Mac will do } a verify after write. I've not found any burner program for the PC } that will verify after write. Strange. } } The IDE drive trays seem like a good approach to backup. The } drives too are obsolete rather quickly. My "new" IBM 45G Deskstar } ATA-66 drives are now discontinued. IBM makes ATA-100 } 45G drives for $239 versus the $129 I paid for the ATA-66 ones. ============= I just use a regular IDE drive it's about as cheap and not much more trouble to change if you put it in the bottom bay and don't screw it in. That works well for me but it would not work well for large images. They just generate too much data. } } My only other backup option (a redundant one) is a Sony SDT-9000 } 4mm DAT. Using native hardware compression, it will store 24G } on a DDS-3 120meter tape. But this has some peculiar problems } based on lack of backup software for tape that works in a dual } host adapter environment. Dantz's Retrospect works great on } the Mac but fails on the PC. I have to use old Win95 Adaptec } backup. It works but does not offer user interface to the } drive's features. ==================== Be careful reusing tapes. They can only be use a few times before they start getting unreliable. One I was using recommended 5 reuses.
Tape is also slow to get a single file from. The one I want is always on the end. } } It seems that as we rush from film to digital, we may look back } on the thousands of negs or chromes sitting in file cabinets } and wonder what happened. We'd now have file cabinets of } $200 hard drives which may or may not work after sitting for } some amount of time. A rather unsettling feeling.
I agree that it is unsettling. That why I have said in the past photographic film is probably still the best archival media we have from cost, aging and resolution point of view. It's fatal flaw is lack of instant availability and knowing if you got a good shot or not while you are still set up.
An interesting setup would be a beam splitter that would let you take either plain old film or CCD images. Then you could do your long term storage on film that we know won't go obsolete with of the next upgrade and we have no questions about how long it will last. Film is competitive or cheaper with digital storage if you include resolution in the equation.
Gordon Gordon Couger gcouger-at-couger.com Stillwater, OK www.couger.com/gcouger 405 624-2855 GMT -6:00
What I have been doing, for convenience more than anything, is to copy my SEM & PM prints with a digital camera at 1024 by 768 resolution. I use a copy stand for its light sources but I hand-hold the camera (!). After all, the images are already at their maximum enlargement, so I won't be looking for more detail than can already be seen in the original image. They print at 200 dpi, not as good as what the printer can do (600 dpi) but they look fine in my reports, and then I can use HTML to write the report because the macro images are in a digital format, too. Extra copies are no longer a problem; in the "good old days" we (Amenex's microscopist, that is) had to spend days at a time making contact prints in a rube-goldberg photo lab set up in the metallographic preparation room (only one that's dark enough).
On the other hand, when one starts making digitally recorded images on the SEM, theoretically one is creating a super-wide-angle image. Does the resolution hold up ? If not, we're kidding ourselves like the fly on a raft who wants the drawbridges raised ...
Best regards, George Langford, Sc.D. amenex-at-amenex.com http://www.amenex.com/
I would greatly appreciate some hints concerning the kind of materials (minerals ?) that could be used in order to determine the k(A,B) (Cliff-Lorimer approx.) factors for my instrument (TEM CM-200 Philips microscope with EDAX EDS X-ray spectrometer) concerning Zr(K-lines), Y(K-lines), Hf(L-lines) and La(?-lines). Do they exist Si containing minerals which could be used to determine the k factors relating Si and the above mentioned elements ? Are they suppliers of standard materials that could be used for determining the k factors for the above mentioned elements ?
Thank you in advance !
Corneliu Sarbu, PhD Dept.of Metallurgy and Applied Materials Science Catholic University of Leuven Belgium
Email: jwahom01-at-tufts.edu Name: Jane Wahome School: Tufts University
Question: I need to view calcium carbonate crystals with a transmission electron microscope for a research project. I also need to record the images. All I've managed to do so far is order thin carbon grids. I have been asked to write a plan for my experiment but I have no clue how to prepare crystals in solution for magnification or what tools to use. Please give me some direction. My professors say I should figure everything out myself - "It will be a good learning experience."
I only do digital images on the SEM. There are several providers of this capability for retrofitting. Some if not most all current SEM makers include digital imaging. When running an active scan system, the digital image is just as on the TV screen and Polaroid output film. But it can be made different. Since the voltage points for limits of the scanned frame are user programmable, a small region can be scanned at very high resolution or a larger region at a lower resolution. The limiting factor is the number of bits in the D/A converter which drives the scan coils. Most of these are 12-bits, so that makes 4096 discrete positions across the X range specified and 4096 discrete positions for the Y range.
My highest recording setting is 4032x2688 pixels which is 10.8M pixels at 8-bits per pixel or twice that at 16-bits per pixel. The 4032x2688 values are chosen to make the aspect ratio 1.5:1, so it fully fits a 35mm frame. The normal 1.33:1 does not. Given that the scan limits are set as for a Polaroid shot, the equivalent pixel density is between 700 and 800 pixels per inch for the digital capture image. Not bad at all. And since the pixel dwell time is programmable, one can optimize it for scan time and minimum noise.
gary g.
At 06:12 AM 1/7/01, you wrote: } Hello Gary, Gordon & Microscopists ! } } [snip] } On the other hand, when one starts making digitally } recorded images on the SEM, theoretically one is creating } a super-wide-angle image. Does the resolution hold up ? } If not, we're kidding ourselves like the fly on a raft } who wants the drawbridges raised ... } } Best regards, } George Langford, Sc.D. } amenex-at-amenex.com } http://www.amenex.com/
----- Original Message ----- } From: "Chris Jeffree" {c.jeffree-at-ed.ac.uk} To: "Gordon Couger" {gcouger-at-couger.com} Cc: {microscopy-at-sparc5.microsocpy.com} Sent: Sunday, January 07, 2001 8:34 PM
George, What do you mean by a super-wide-angle picture? The digital scan output goes through the mag control, so your angle is the same as for Polaroid at a given mag. The resolution is determined by the pixel density and won't exceed a Type 55 negative on your ETEC until you capture about 4k by 4k. 2k by 2k isn't quite as good as you can do with film, the limiting factor being your record CRT and camera. As Gordon said, film is still the measure. It lasts, the resolution is great and software "upgrades" won't make your entire file obsolete.
Besides, don't you have some problems using pure digital imaging for legal cases? My understanding is that if you use digital, the original file must be on a WORM drive (now known as CD-R) to give the equivalent of an original negative on file. This info came from the Virginia Crime Labs quite a few years ago.
Ken Converse, owner Quality Images Delat, PA
George Langford, Sc.D. 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 Gary, Gordon & Microscopists ! } } What I have been doing, for convenience more than anything, } is to copy my SEM & PM prints with a digital camera at 1024 } by 768 resolution. I use a copy stand for its light sources } but I hand-hold the camera (!). After all, the images are } already at their maximum enlargement, so I won't be looking } for more detail than can already be seen in the original } image. They print at 200 dpi, not as good as what the printer } can do (600 dpi) but they look fine in my reports, and then } I can use HTML to write the report because the macro images } are in a digital format, too. Extra copies are no longer a } problem; in the "good old days" we (Amenex's microscopist, } that is) had to spend days at a time making contact prints } in a rube-goldberg photo lab set up in the metallographic } preparation room (only one that's dark enough).
} } On the other hand, when one starts making digitally } recorded images on the SEM, theoretically one is creating } a super-wide-angle image. Does the resolution hold up ? } If not, we're kidding ourselves like the fly on a raft } who wants the drawbridges raised ... } } Best regards, } George Langford, Sc.D. } amenex-at-amenex.com } http://www.amenex.com/ } } }
} What do you mean by a super-wide-angle picture? The digital scan } output goes through the mag control, so your angle is the same as } for Polaroid at a given mag. The resolution is determined by the } pixel density and won't exceed a Type 55 negative on your ETEC } until you capture about 4k by 4k. 2k by 2k isn't quite as good as } you can do with film, the limiting factor being your record CRT and } camera.
The image I see on the Polaroid film comes nowhere near taxing the resolution of the film. My 1024 by 768 pixel digicam snapshots of the original Polaroid prints look pretty close to the originals. Why enlarge them any more ? Empty magnification and all that. Yes, I know that the twelve- or sixteen-bit ADC's can capture a much wider range of exposure than can film, but I don't see where all those pixels get us any more spatial resolution. A 35 mm camera can cram a lot of resolution onto a small area of film, but its lens is reducing the original scene, not enlarging it. All the fancy lenses on our metallographs can't do any better than covering the 4X5 inch format of the film at maximum resolution. If we try to use a smaller eyepiece to get a wide-angle effect, then the edges of the image show terrible distortion. So there's no point in using an excessive number of pixels to describe the output of a microscope's imaging system.
} As Gordon said, film is still the measure. It lasts, the } resolution is great and software "upgrades" won't make your entire } file obsolete.
Isn't it the hardware that goes South ? Where do I read my eight-inch floppies; or the 5-1/4 inch ones, for that matter ... ? Once a bit map, always a bit map, I should think. I do notice that my .JPG image editor can't make heads or tails of some of the .JPG files that look fine on Netscape, so there are some software issues, but it looks as though the old drives are the real problem.
} Besides, don't you have some problems using pure digital imaging } for legal cases? My understanding is that if you use digital, the } original file must be on a WORM drive (now known as CD-R) to give } the equivalent of an original negative on file. This info came from } the Virginia Crime Labs quite a few years ago.
I lock the original floppy disk and leave the original image files untouched there. Then I copy 'em to my hard drive for cropping and adjustment of contrast, etc. Anyone wants to see the report, gets the whole shebang: originals, thumbnails, edited pix, and text (HTML). CDROM's are handy for the monster files that result. One report had almost a thousand individual files in it. Client wasn't too happy with the task of learning what a browser is. Printing it all out is a monumental PIA, but then, so is ruffling through a two-inch-thick pile of prints.
Best regards, George Langford Principal Consultant Amenex Associates, Inc. http://www.amenex.com/
I can assure you all that TAAB is well and truly still in business as we communicate on a regular basis concerning cryostats and microtomes. Please contact TAAB on: sales-at-taab.co.uk
Best. Regards
Alan Bright
Bright Instrument Co.Ltd. St Margaret's Way Huntingdon Cambridgeshire PE29 6EU England
Tel No:+44 (0)1480 454528 Fax No:+44 (0)1480 456031 Email: AlanBright-at-brightinstruments.com Web Site: www.brightinstruments.com
-----Original Message----- } From: Roger Moretz [mailto:rcmoretz-at-excite.com] Sent: 05 January 2001 13:29 To: Patton, David; Brownell, Patrick Cc: 'Microscopy-at-MSA.Microscopy.Com'
Patrick:
I don't know the machine, but is TAAB no longer in business in the UK? For the longest time TAAB supplies (altho not generally easily available in the US) was an excellent source of resins and small items. Regardless, I would think that the worn rubber pad is your problem. Again, thinking of experience with other knifemakers, the pads are an essential part of relieving some of the stress in the glass as it breaks. If this pad is uneven, it may not be absorbing the pressure/stress as it should. Perhaps (if TAAB is not around) some other users of the knifemaker might have accessories (like a spare pad) to help you out. Also check the following: depth of the score--if it's too deep or too light, that will affect the break and edge quality; how fast are you breaking after scoring? - a slow break has always been essential to consistently good knife edges for me; check the setting of the clamp(s) and pressure points to ensure that there are no uneven points and that the clamp(s) are providing equal pressure. I can't find the reference right now, but the original publications on making the Ralph knives by hand (it was in Stain Technology, I think) might get you by, and it also might allow you to check the quality of the glass. The technique wasn't too difficult or tedious, and, as I remember (from the dim recesses of ancient history) the percentage of good knives was acceptable. Hope this helps.
Roger Moretz, Ph.D. Dept of Toxicology Boehringer Ingelheim Pharmaceuticals, Inc.
On Fri, 5 Jan 2001 09:21:24 +0000 (GMT Standard Time), Patton, David 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 } -----------------------------------------------------------------------. } } } Perhaps you could get a lab with no problems to make some } knives with your glass and then test them in their lab and } yours (get them to send some of their glass to you as } well to test your knifemaker). That should show if it is } the glass, the knifemaker or the ultramicrotome that is at } fault. } } Dave } } } On Wed, 3 Jan 2001 08:04:10 -0800 "Brownell, Patrick" } {patrick.brownell-at-weyerhaeuser.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 } } -----------------------------------------------------------------------. } } } } } } My problem is a poor knife edge. The knife looks fine under casual } } observation, or with small magnification, but when it comes time to actually } } do some sectioning, I get a lot of chattering, or streaking, or both. I } } know make as many test blocks as I do sample blocks, so I don't waste } } samples with all the bad glass knifes. I've gone through several boxes of } } glass over the past two months, and only get a useable knife every 15 to 20 } } breaks. The same knife breaker has worked fine in the past, and I have } } changed the scoring wheel, and checked all that I can. } } } } This knife breaker is also very hard to get parts for. The only obvious } } problem is that one of the pressure points has a rubber pad that is unevenly } } worn. I don't see how that would cause my problem. Again, the knifes look } } good to the naked eye. } } } } The glass I use is from Electron Microscopy Sciences. They are called ultra } } glass knife strips 6.5mm x 25mm x 400 mm. } } } } I guess I'm just looking for someone who has had a similar problem, and } } fixed it in some manner. Could I have gotten a bad batch of glass? I don't } } think it is very likely, I've used several boxes, but they may all be from } } the same batch, for all I know. Is there another brand of glass, or breaker } } that others have found produce reliable knives? } } } } Thanks for any and all help } } } } -Patrick Brownell } } } ---------- } } } From: Katja M. Wolski[SMTP:kwolski-at-hsc.usf.edu] } } } Reply To: kwolski-at-hsc.usf.edu } } } Sent: Wednesday, January 03, 2001 4:26 AM } } } To: Brownell, Patrick } } } Subject: Re: Ralph Glass Knife problems } } } } } } I use a different knife machine, but what's the problem you're having? } } } Are you } } } not getting a good knife edge or what? } } } } } } Katja } } } } } } } } } } } } "Brownell, Patrick" 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 use Ralph type glass knives for plastic sectioning of biological } } } samples. } } } } I am experiencing problems in making a proper knife. I have a TAAB } } } } histoknifemaker (also says Reichart-Jung). Is there anyone willing to } } } offer } } } } expertise in this area? } } } } } } } } -Patrick Brownell } } } } } } } ---------------------------------------- } Patton, David } Email: David.Patton-at-uwe.ac.uk } "University of the West of England" } }
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We are using Magneto-Optical Disks, 2.6 or 5.2 Gb to store the data. They are very reliable (manufacturer claims, that data may be stored up to 50 years) it's not sensitive for magnetic fields and heat (in reasonable temperature diapason, actually until melted). You may rewrite data many times (a million, I believe). Because of reliability, US government uses this media to store all digital data. MO disk needs special drive, which suppose to be connected to the computer (to the PC in our case, SCSII). It's connected to the network, so it is accessible from other computers. We have to insert/remove MO disk by hands of coarse. 2.6 Gb MO is about $40-80 each. MO drive - about $1000. I am not so happy with this instrumentation (relatively slow, but faster than CD or Zip-drive, you have to have special MO-drive connected to the particular computer etc), but it's only known to me a media, which is reliable: CDR/CDRW - absolutely not reliable, light-sensitive, etc.; Zip-drive/diskette is not enough for me, HD- not bad idea, but technically not that easy (you have to have removable HD, I did have a problem with that setup when WinNT changed the letters to the logical drives and therefore all my programs suddenly stopped when I removed the HD, and you have to restart the computer if you want to remove HD). Currently, I do have approximately 10 Gb data stored on MO disks. In our Department there are 200 or so disks are in use. To my knowledge we did have one case when MO disk virtually lost the data but all 100% data has been recovered later. Something like that may happens if you will try to remove the disk during the writhing (what, probably was happens). If I am going to work with some block of data, I copied that to the server and work on it from any computer even from home. The same happens with fresh portion of data: I temporary store the data on the server and then (after frequent reminding from SysAdmin), transfer it to the MO disk. It takes approximately 20 min to transfer 1 Gb of data. Detailed information about MO disks you may find on the Internet.
To help improve the reliability of ZIP disk there is a freeware program available from Gibson Research, TIP.exe . see http://www.grc.com
At 08:16 PM 1/5/01, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
} } And there were all those Zeiss microscopes in Jurassic Park. Pity the one } they were using in one scene (an Axiophot?) didn't have a condenser.... } And let's not forget the Cambodian lady in "Blade Runner" (1982) who operates an SEM in the street (in the rain!!?). She helps Harrison Ford identify a scale in evidence as having come from a bioengineered snake, not a fish (bioengineered animals apparently have serial numbers on even their smallest parts). There was another, more recent movie called "Mimic" in which there is a scene where an insect specialist has a pile of SEM micrographs on her desk, purportedly representing various insect eggs or larvae. As a former micropaleontologist, I could tell they were actually illustrations of planktonic Foraminifera, but I suspect this distinction was lost on much of the viewing public.
Frank Thomas Geological Survey of Canada Bedford Institute of Oceanography Dartmouth, Nova Scotia Canada
I have done a lot of EM on ZnO and CaCO3 crystals a while ago. I simply made a suspension of the powder in ethanol or methanol and ultrasonicated them for 3 to 5 min. I then just dropped one or two drops of the suspension on the grid positioned on a filter paper and let it dry. You might want to check with the SEM that you do not change morphologies by the ultrasound treatment. I suggest that you first take some SEM images anyway to get some information on sizes, distributions and morphologies. IF you have rather large crystals. SEM will not work, if the crystals are too small. In that case you will have to go directly to the TEM. If you are taking the crystals directly from a reaction solution, just give a drop or two on the grid and let dry. Of course in that case, you might also have non CaCO3 material on the grid depending on your reaction. You will have to make sure that you are looking at the CaCO3 and not some other crap. This can be done by electron diffraction or HRTEM. Image recording possibilities depend on your microscope. What microscope are you using ? If you need further information or want to discuss some things feel free to send an email.
Andreas
************************************************* Dr. Andreas Taubert Materials Science and Engineering Dept. 3231 Walnut Street The University of Pennsylvania Philadelphia PA 19104-6272 tel: +1 215 898 2700 fax: +1 215 573 2128
Physical Chemistry is everything for which 1/T is linear ... *************************************************
----- Original Message ----- } From: {jwahom01-at-tufts.edu} To: {Microscopy-at-sparc5.microscopy.com} Sent: Sunday, January 07, 2001 11:23 AM
Or not. I guess I just can't ignore this thread. I have always been vocal about inconsistencies/stupidities/errors in TV/movies/etc. So, as to Andromeda Strain: first of all, there was the insertion of the specimen without use of an airlock (and those of us who suffered with the Forgflo/nee RCA EMU-4 know that the beast had this horrid airlock that used the external bellows minipump!!!); then there was the immediate location of the desired area under the beam....; plus all those already mentioned. On Quincy: the first episode (or maybe 2) the lab was fully outfitted with Zeiss equipment; the rest of the series the lab was outfitted with AO (must be nice to have that kind of equipment budget--but why go that direction??? could it be politics???); then the SEM/microprobe episode, where, once again, the area of interest with the decisive inclusion was magically right in the area being examined immediately; then there was the TEM episode where Sam received the biopsy about 4am and had a block, stained sections and a confirmatory diagnosis by 8am (now there's a reality check for you--did your boss pick up on that and demand that turn-around for you????); I'm sure there were others but those stuck (mostly in my craw). And a final overall plaint about the fact that everybody was working (at high mag, no less) in brightly lit rooms, when we toiled away in near pitch dark!! Even that Forgflo/RCA with its ma beam current couldn't do that--I know from many hours in the dark, dark adjusting my eyes.
O well, as someone put it--that's Hollyweird.
Roger Moretz Ph.D. Dept of Toxicology Boehringer Ingelheim Pharmaceuticals, Inc. On Sat, 06 Jan 2001 11:19:43 -0800, Robert Ruscica 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 have enjoyed reading all the TV trivia regarding the Quincy and Andromeda } Strain. What many of you may not know is that for the "Strain" movie the } makers of the film contacted a now defunct Microprobe Company, Materials } Analysis Co. We sent to the studio an Electron Microprobe. The only portion } that made the film was some blinking x-ray scalers and a portion of the } electronics rack. What the impact of microprobe was in the film I can't } guess or remember. } In the Quincy episodes, there were more than one, we sent to the studio an } ISI SEM along with a service engineer, whose name at the moment escapes } me, to install it and our application and Demonstration man, Bill Roth to } run the SEM, Bill has been with Hitachi for many years now and could give
} more incite as to what happened at the studio than I can as he was there } for a week doing the one episode. I remember him telling me that Quincy's
} technician, Sam was explaining to Quincy what was on the CRT with the } camera going from the control panel with Bill's hands being filmed but the } overall shot of Sam and Quincy looking at the CRT and discussing the } forensic material. I still have some 8x10's around here somewhere of the } filming. Thought you might be interested. } } Regards, } Bob Ruscica } }
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I need some assistance in making up a uranyl acetate stain. I have powdered uranyl acetate and would like to know what concentration and solvent to use to make a good stain for looking at meat samples in the TEM. If there are any procedures (time and temp) that I should adhere too that would also be much appreciated.
Ps. I'm microtoming the TEM samples first then applying the uranyl acetate stain with a follow-up stain of RuO4 vapor.
thanks all dz
David Ziegler U.S. Army, SBCCOM AMSSB-RSS-MS(N) Materials Science Team, SS&T Natick, MA 01760-5020 TEL: (508) 233-6484 FAX: (508) 233-5521 Email: David.Ziegler-at-Natick.Army.Mil
Gatan, Inc the technology leader in digital imaging, analytical spectroscopy and ion beam milling applications for electron microscopy is seeking candidates for an Analytical Product Manager. This person will manage the complete product life cycle for this company's product line. Responsibilities include coordinating all activities necessary to achieve the strategic revenue and profit objectives for the product. For the Product manager there are three key product cycle phases: 1) Planning: includes market research, Marketing plan production and results in a vision statement to pass to development. This the key stage in the development of any new product. The vision statement is the marketing vision for the product and it may include an analysis of competitor's products and a projection of opportunities in the future. 2) Development: Pricing, product positioning, product packaging and product promotion.3) Stabilization: Beta testing, code testing and feedback to developers and product launch. The applicant must have significant product management experience, preferably in a product area that is applicable to market: TEM applications, electron microscopy, biological, materials or semiconductor experience would be useful. Familiarity with existing vendors, consultants, competitors, etc in the industry is a plus. Technical knowledge of Gatan software and hardware applications. A proven track record in both planning and executing successful product management programs. Must be comfortable with current development environments and development tools to work intelligently with engineering. Must have excellent overall PC computing skills, including a thorough familiarity with market tools in document composition, database design and presentation management. MBA preferred; PHD desired with a background in TEM and experience with GIF and PEELS systems. Salary: Base salary plus bonus commensurate with experience. Interested candidates should send email or fax their resume to:
GATAN, INC Attn: HR Department 5933 Coronado Lane Pleasanton, CA. 94588 Fax: (925) 463-0204 Email: hr-at-gatan.com www.gatan.com
Carlotta Daniels GATAN, Inc. Human Resources Pleasanton, CA. 94583
there are also a number of follow-up links, which I have not explored.
The latter link has the following section:
So, How Long Can CDs Last? Leaving aside scratches, fires, floods, and peanut butter sandwiches and concentrating on the slow chemical changes that determine the inherent life expectancy of a CD, extensive accelerated-aging tests suggest that Kodak writable CD products, including Photo CD discs, will not reach a BLERmax of 50 for a period of around 200 years when kept in the dark at moderate storage conditions. This long potential life expectancy is mainly a function of the greater dark stability of the dye used in Kodak writable CD products. Considering that BLERmax 50 is still not an unreadable level of error, Kodak writable CDs have a very long life expectancy indeed. Similar research by the 3M Company shows that CD-ROM products made by them will not attain a block error rate of 50 per second for more than 100 years in moderate storage conditions.
Accelerated aging is subject to uncertainties, but it does rest on firm scientific footing. Behind the data is the simple assumption that raising the temperature causes the reactions of decay to happen faster--so fast, in fact, that they occur within a few months, rather than decades. The science of reaction rates is called kinetics, and the lifetime predictions are based on well-established principles of that branch of chemical science. These same principles are used every day to design the chemical plants and processes of the modern world. Because there is so much practical experience with the laws of kinetics, lifetime predictions based on them are approximately correct. Such test methods soon will be part of a forthcoming ANSI (American National Standards Institute) standard dealing with tests for CD permanence.
End of citation.
So, from a scientific standpoint (accelerated aging), a good writeable CD should have a lifespan of 100-200 years, which is more than tape (several decades) and on par with film, at least as far as I can tell. Film suffers from the same problems the CD suffer from (sensitivity to light, scratches, fire, alien attacks, etc.).
Finally a few words regarding M/O and CD:
We supplied with our systems until a few years ago an M/O drive. At that time, there were only CD-ROMs. The drives were (are?) fairly expensive, about $1000 for the drive, and with the advent of cheap CD-Rs it became harder and harder to find drives and media. The drives are much more common in Europe. In addition, the drives are pretty slow, and it was always a hassle to work with the drives under Windows NT. The drives use a laser to heat the storage medium, then a magnetic head to write the info to the heated patch. This might result in a more stable storage than CD or magnetic. The availability, however, seems to be a big problem.
Michael
Michael Bode, Ph.D. Soft Imaging System Corp. 1675 Carr St., #105N Lakewood, CO 80215 =================================== 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: Sergey Ryazantsev [mailto:sryazant-at-ucla.edu] Sent: Monday, January 08, 2001 4:08 AM To: microscopy-at-sparc5.microscopy.com
Hello,
We are using Magneto-Optical Disks, 2.6 or 5.2 Gb to store the data. They are very reliable (manufacturer claims, that data may be stored up to 50 years) it's not sensitive for magnetic fields and heat (in reasonable temperature diapason, actually until melted). You may rewrite data many times (a million, I believe). Because of reliability, US government uses this media to store all digital data. MO disk needs special drive, which suppose to be connected to the computer (to the PC in our case, SCSII). It's connected to the network, so it is accessible from other computers. We have to insert/remove MO disk by hands of coarse. 2.6 Gb MO is about $40-80 each. MO drive - about $1000. I am not so happy with this instrumentation (relatively slow, but faster than CD or Zip-drive, you have to have special MO-drive connected to the particular computer etc), but it's only known to me a media, which is reliable: CDR/CDRW - absolutely not reliable, light-sensitive, etc.; Zip-drive/diskette is not enough for me, HD- not bad idea, but technically not that easy (you have to have removable HD, I did have a problem with that setup when WinNT changed the letters to the logical drives and therefore all my programs suddenly stopped when I removed the HD, and you have to restart the computer if you want to remove HD). Currently, I do have approximately 10 Gb data stored on MO disks. In our Department there are 200 or so disks are in use. To my knowledge we did have one case when MO disk virtually lost the data but all 100% data has been recovered later. Something like that may happens if you will try to remove the disk during the writhing (what, probably was happens). If I am going to work with some block of data, I copied that to the server and work on it from any computer even from home. The same happens with fresh portion of data: I temporary store the data on the server and then (after frequent reminding from SysAdmin), transfer it to the MO disk. It takes approximately 20 min to transfer 1 Gb of data. Detailed information about MO disks you may find on the Internet.
} } Could someone post the reference for the article for making glass knives } by hand?
Here's the original reference, which includes a bit of the history of Ralph knives (in honor of the late Dr. Paul Ralph): Stain Technology 51(2): 71-97. [1976]. Bennet et al. Science and art in preparing tissues embedded in plastic for light microscopy, with special reference to glycol methacrylate, glass knives and simple stains.
Good luck. Mike Nesson _______________________________________________________________________ Michael Nesson, Ph.D. Department of Biochemistry & Biophysics 2011 Ag&LS, Oregon State University, Corvallis, OR 97331-7305 (541)737-5245 FAX:(541)737-0481 nessonm-at-ucs.orst.edu
Out here in Sunny Southern California we just purchased a AMT 1K digital camera for use in our EM lab at the UCLA Medical Center. The storage device or choice for archiving we utilize is to burn CD's of the images as long term storage.
=========== } } Just a word of caution about Zip disks. They can be very } } unreliable. When Iomega first came out with them, their } } media was really good. Now it is not the same. Maxell } } and Fujifilm also make media. I think that theirs are better. } } } } The other problem with Iomega drives (Zip and Jaz) is the } } click of death. This is a precursor to a dead drive or } } media and loss of all that is on the media (if bad media). } } } } To check your drives and media, run tip.exe. To find out } } more about this, visit http://www.grc.com } } } } gary g. } } Gary, } } Zip files not Zip disk. Use Pkzip or some other program to put all the } files into one zip file, usually a complete directory, copy that file to } the back up media and verify the zip file on the back up media. Currently } I use write only CD-ROMs and keep a copy of really important stuff on my } internet server at my ISP as well. Hard disk space is cheap. I have the } last 15 years work at my finger tips. If I can find it:) I started using } this on single sided single density floppies on a Radio Shack Model 1. I } can only think of two times that I was unable to retrieve a file in 20 } years. } } I am a programmer not a photographer so a years work might fit on a floppy } disk. } } I am not satisfied with the life of CD-ROMs but so far something better } has always come along before the old media went bad and I copied it all } over. One thing I don't like about CD-ROMs is they are not protected from } scratching or being broken. } } Gordon } Gordon Couger gcouger-at-couger.com } Stillwater, OK www.couger.com/gcouger } 405 624-2855 GMT -6:00 }
On the HP CD Writer there are two programs for writing to a CD.. Out here we use the CD-R one time write to the disc.
There is the HP program for writing a CD which does not have a way to verify the CD was written. There is also another program that comes with the CD writer from HP that performs a write speed test on the disc then writes to the disc and then it verifies the disc... the program is called MY CD on the HP CD writers....
How may I calculate (OK, make an educated guess) the temperture on my grid in the TEM? I know it depends on the high voltage, the beam current, the thickness of the specimen, the contact between grid and holder, and the phase of the moon, and so probably I won't *really* know. All I need is a ballpark figure, like is it 80C or 200C or 1500C?
I'm watching something presumably melt and fuse/crystallize on my LEO 912 EFTEM at 100-120 kV with a beam current of somewhere in the neighborhood of 10 uA. This is not necessarily a bad thing - it tells me something useful about these Si nanoparticles!
Mahalo, Tina
Sunny, clear, about 74F, South Shore flat, North Shore up.
**************************************************************************** * Tina (Weatherby) Carvalho * tina-at-pbrc.hawaii.edu * * Biological Electron Microscope Facility * (808) 956-6251 * * University of Hawaii at Manoa * http://www.pbrc.hawaii.edu/bemf* ****************************************************************************
How may I calculate (OK, make an educated guess) the temperture on my grid in the TEM? I know it depends on the high voltage, the beam current, the thickness of the specimen, the contact between grid and holder, and the phase of the moon, and so probably I won't *really* know. All I need is a ballpark figure, like is it 80C or 200C or 1500C?
I'm watching something presumably melt and fuse/crystallize on my LEO 912 EFTEM at 100-120 kV with a beam current of somewhere in the neighborhood of 10 uA. This is not necessarily a bad thing - it tells me something useful about these Si nanoparticles!
Dear Tina, I posted something similar to the list a while ago, and wrote up a more complete version for Microscopy Today. Although the variables are different, the technique should be the same. A number you'd need would be the stopping power of Si for 100 kV e-, which is 3.274 Mev cm^2/gm. The radiative stopping power is much smaller than the collisional stopping power, which is 3.265 MeV cm^2/gm (since the radiation should escape the particle, use this latter number). Use this to calculate how much energy is transmitted to the specimen for each electron by multiplying the stopping power by the density of Si (2.33 gm/cm^3) to get how much energy is deposited per unit path length, figuring out the path length of each electron, and using the beam current flux (in e-/nm^2 or the like) to get how many e- strike the particle each second. Next, calculate the heat losses by conduction and radiation as a function of temperature, and the steady-state temperature of the specimen--the number you want--will be where the heat absorbed is equal to the heat lost. I assumed that heat radiated and that conducted from the immediate vicinity of the particle would be lost in an essentially infinite heat sink, and that the moon was in third quarter.
Sunny, clear, about 74F, South Shore flat, North Shore up.
Cloudy, about 270 K, Hudson icy. Yours,
Bill Tivol Wadsworth Center Albany NY (518) 473-7399 WFT02-at-health.state.ny.us
Two minerals are fairly easy to come by Zircon (SiZrO4) and Hafnon (SiHfO4) or could be synthesized. The rare-earth elements more commonly form phosphate minerals such as monazite ((Light REE)PO4) and xenotime ((Heavy REE,Y)PO4). The substitution of Huttonite (SiThO4) into these structures would allow for the calculation of REE,Y/Si k-factors. The problem with these minerals is that they are normally not homogeneous, so special care must be made to correlate electron microprobe with TEM analyses. Alternatively, you could try to synthesize your own standards. Hope this helps, Ken } } Hi, everybody ! } } I would greatly appreciate some hints concerning the kind of materials } (minerals ?) that } could be used in order to determine the k(A,B) (Cliff-Lorimer approx.) } factors for my instrument } (TEM CM-200 Philips microscope with EDAX EDS X-ray spectrometer) concerning } Zr(K-lines), } Y(K-lines), Hf(L-lines) and La(?-lines). Do they exist Si containing minerals } which could be } used to determine the k factors relating Si and the above mentioned elements ? } Are they suppliers of standard materials that could be used for determining } the k factors for the } above mentioned elements ? } } Thank you in advance ! } } Corneliu Sarbu, PhD } Dept.of Metallurgy and Applied Materials Science } Catholic University of Leuven } Belgium
Around 20 years ago, I saw a movie about killer bats in which, after looking at a slide with what looked like a Tasco microscope, the scientist exclaimed "It's just as I feared - the rabies bacillus!". To add insult to injury there followed a view through the microscope where, if I recall correctly, a paramecium was swimming.
It's my understanding that dye-based CD-ROMs aren't archival, but the gold-based version is. Anyone know more about this?
Dee
*************************************************************** Dee Breger Mgr. SEM/EDX Facility Lamont-Doherty Earth Observatory 61 Route 9W Palisades, NY 10964 USA T: 914/365-8640 F: 914/365-8155
http://www.ldeo.columbia.edu/micro http://www.discovery.com/area/science/micro/micro1.html http://www.lsc.org/antarctica/front.html Journeys in Microspace (Columbia University Press, 1995)
sorry for bothering you with that. I wanted to send an email to Phil Oshel, but deleted the email before writing down his email address. Phil, please contact me off-list, thanks.
Andreas
************************************************* Dr. Andreas Taubert Materials Science and Engineering Dept. 3231 Walnut Street The University of Pennsylvania Philadelphia PA 19104-6272 tel: +1 215 898 2700 fax: +1 215 573 2128
Physical Chemistry is everything for which 1/T is linear ... *************************************************
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Reply to: Re: Ultimate and perhaps last of TV Trivia Dear All,
I too have been enjoying this conversation and thought I would sit back and read. However, I can't resist a few comments. After all we have one of the actual Zeiss microscopes from Jurassic Park in our lab. It works wonderfully, as a Zeiss microscope should. The only madification they made was to paint it pink to look right on film. Being so close to Hollywood, we have a few other pieces of famous furniture around the lab. I must admit that I too look out for appearances of microscopes, and especially EM's in the media, but I think I must be a little more tolerant of the way we are portrayed. My phylosophy is that as long as we are out there, then it is a good thing. Who cares if the portrayal is accurate or not, we can sort that out in our lectures. At least we are being recognized. After all, it is much better to be talked about (no matter the subject) than to be ignored.
If we systematically went through film portrayals of any subject then I am sure we will find Hollywood had managed to insult just about every scientific disipline, ethnic group and foreign country. Who cares, its only entertainment. Watch out instead for the school science books that show cells with organelles but do not show the Golgi complex, or the histology books that omit the lysosomes. They are there. This is far more harmful to the scientific community.
I enjoyed the comments from Roger Moretz about the speed samples are processed. After all one of the roles of this form of entertainment has become a predictor of the future. Maybe the portrayals are so so inaccurate after all. We already work with microscopes in full daylight (from computer screens), we are close to having 4hr sample processing for resin-embedded samples (cf microwave processing), and we can already section and examine biopsies in less than 2 hr (with cryosectioning methods). Two thumbs up for Hollywood for showing us the way.
Paul Webster.
Paul Webster, Ph.D House Ear Institute 2100 West Third Street Los Angeles, CA 90057 phone:213 273 8026 fax: 213 413 6739 e-mail: pwebster-at-hei.org http://www.hei.org/htm/aemi.htm
Roger Moretz wrote:
} Or not. I guess I just can't ignore this thread. I have always been vocal } about inconsistencies/stupidities/errors in TV/movies/etc. So, as to } Andromeda Strain: first of all, there was the insertion of the specimen } without use of an airlock (and those of us who suffered with the Forgflo/nee } RCA EMU-4 know that the beast had this horrid airlock that used the external } bellows minipump!!!); then there was the immediate location of the desired } area under the beam....; plus all those already mentioned. On Quincy: the } first episode (or maybe 2) the lab was fully outfitted with Zeiss equipment; } the rest of the series the lab was outfitted with AO (must be nice to have } that kind of equipment budget--but why go that direction??? could it be } politics???); then the SEM/microprobe episode, where, once again, the area } of interest with the decisive inclusion was magically right in the area } being examined immediately; then there was the TEM episode where Sam } received the biopsy about 4am and had a block, stained sections and a } confirmatory diagnosis by 8am (now there's a reality check for you--did your } boss pick up on that and demand that turn-around for you????); I'm sure } there were others but those stuck (mostly in my craw). And a final overall } plaint about the fact that everybody was working (at high mag, no less) in } brightly lit rooms, when we toiled away in near pitch dark!! Even that } Forgflo/RCA with its ma beam current couldn't do that--I know from many } hours in the dark, dark adjusting my eyes. } } O well, as someone put it--that's Hollyweird. } } Roger Moretz Ph.D. } Dept of Toxicology } Boehringer Ingelheim Pharmaceuticals, Inc. } On Sat, 06 Jan 2001 11:19:43 -0800, Robert Ruscica 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 have enjoyed reading all the TV trivia regarding the Quincy and } Andromeda } } Strain. What many of you may not know is that for the "Strain" movie the } } makers of the film contacted a now defunct Microprobe Company, Materials } } Analysis Co. We sent to the studio an Electron Microprobe. The only } portion } } that made the film was some blinking x-ray scalers and a portion of the } } electronics rack. What the impact of microprobe was in the film I can't } } guess or remember. } } In the Quincy episodes, there were more than one, we sent to the studio } an } } ISI SEM along with a service engineer, whose name at the moment escapes } } me, to install it and our application and Demonstration man, Bill Roth } to } } run the SEM, Bill has been with Hitachi for many years now and could give } } } more incite as to what happened at the studio than I can as he was there } } for a week doing the one episode. I remember him telling me that Quincy's } } } technician, Sam was explaining to Quincy what was on the CRT with the } } camera going from the control panel with Bill's hands being filmed but } the } } overall shot of Sam and Quincy looking at the CRT and discussing the } } forensic material. I still have some 8x10's around here somewhere of the } } filming. Thought you might be interested. } } } } Regards, } } Bob Ruscica } } } } } } } } } } _______________________________________________________ } Send a cool gift with your E-Card } http://www.bluemountain.com/giftcenter/ } } } } } } RFC822 header } ----------------------------------- } } Received: from ultra5.microscopy.com [206.69.208.10] by mailhouse.hei.org } with ESMTP } (SMTPD32-6.00) id AC703E6C025E; Mon, 08 Jan 2001 16:33:52 -0800 } Received: (from daemon-at-localhost) } by ultra5.microscopy.com (8.9.3+Sun/8.9.1) id JAA13624 } for dist-Microscopy; Mon, 8 Jan 2001 09:16:16 -0600 (CST) } Received: from no_more_spam.com (sparc5 [206.69.208.10]) } by ultra5.microscopy.com (8.9.3+Sun/8.9.1) with SMTP id JAA13616 } for "MicroscopyFilteredEmail-at-msa.microscopy.com"; Mon, 8 Jan 2001 } 09:15:46 -0600 (CST) } Received: from ewey.excite.com (ewey-rwcmta.excite.com [198.3.99.191]) } by ultra5.microscopy.com (8.9.3+Sun/8.9.1) with ESMTP id JAA13608 } for {Microscopy-at-sparc5.microscopy.com} ; Mon, 8 Jan 2001 09:15:34 -0600 (CST) } Received: from spike.excite.com ([199.172.152.97]) by ewey.excite.com } (InterMail vM.4.01.02.39 201-229-119-122) with ESMTP } id {20010108151408.VOMO24504.ewey.excite.com-at-spike.excite.com} ; } Mon, 8 Jan 2001 07:14:08 -0800 } Message-ID: {18272603.978966848378.JavaMail.imail-at-spike.excite.com} } Date: Mon, 8 Jan 2001 07:14:07 -0800 (PST) } From: Roger Moretz {rcmoretz-at-excite.com} } To: Robert Ruscica {ruscica-at-etp-usa.com} , Microscopy-at-sparc5.microscopy.com } Subject: Re: Ultimate and perhaps last of TV Trivia } Mime-Version: 1.0 } Content-Type: text/plain; charset=us-ascii } Content-Transfer-Encoding: 7bit } X-Mailer: Excite Inbox } X-Sender-Ip: 63.80.54.82 } Errors-to: Microscopy-request-at-sparc5.microscopy.com } X-RCPT-TO: {pwebster-at-hei.org} } X-UIDL: 273278772 } Status: U }
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They are all dye-based. What is silver or gold is the coating on the top of the media. It ca readily be flaked off.
With the metal coating removed, the media is generally transparent. Some have a blue tint while others have little color. Others might look green. But essentially, they are all chalgocencide technology. Some are better than others.
gg
At 03:49 PM 1/8/01, you wrote:
} Colleagues, } } It's my understanding that dye-based CD-ROMs aren't archival, but the } gold-based version is. Anyone know more about this? } } Dee } } } } *************************************************************** } Dee Breger } Mgr. SEM/EDX Facility } Lamont-Doherty Earth Observatory } 61 Route 9W } Palisades, NY 10964 USA } T: 914/365-8640 } F: 914/365-8155 } } http://www.ldeo.columbia.edu/micro } http://www.discovery.com/area/science/micro/micro1.html } http://www.lsc.org/antarctica/front.html } Journeys in Microspace (Columbia University Press, 1995)
These are found all of the time in Hollywood. They are stand-ins. Only a very sharp eye can tell the difference. Notice how well Antonio Banderas dances in "The Mask of Zorro?" Real, or a stand-in? duh.
gary
At 03:49 PM 1/8/01, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Hi Tina, I'm sure this question has been asked before, (look in the archives) - but I think the basic answer is 'it depends'(!). I am currently having terrible trouble with plucked FIB sections of Au metallised GaAs on holey carbon films; the metal melts, alloys with and destroys my specimen even at relatively low beam currents in my JEOL 120 CX. I have been told by our theory guys that little heat will escape by radiation below about 500C, so if you have a sample with very poor thermal conductivity it will be easy to get to this temperature. You may be able to avoid the problem somewhat by using higher accelerating voltages (less inelastic interaction with the specimen, I believe) and/or adding a carbon coating to the specimen to increase thermal conductivity.
Good luck!
Richard
} ------------------------------------------------------------------------ } 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 } -----------------------------------------------------------------------. } } } Happy New Year to you all! } } How may I calculate (OK, make an educated guess) the temperture on my grid } in the TEM? I know it depends on the high voltage, the beam current, the } thickness of the specimen, the contact between grid and holder, and the } phase of the moon, and so probably I won't *really* know. All I need is a } ballpark figure, like is it 80C or 200C or 1500C? } } I'm watching something presumably melt and fuse/crystallize on my LEO 912 } EFTEM at 100-120 kV with a beam current of somewhere in the neighborhood } of 10 uA. This is not necessarily a bad thing - it tells me something } useful about these Si nanoparticles! } } Mahalo, } Tina } } Sunny, clear, about 74F, South Shore flat, North Shore up. } } **************************************************************************** } * Tina (Weatherby) Carvalho * tina-at-pbrc.hawaii.edu * } * Biological Electron Microscope Facility * (808) 956-6251 * } * University of Hawaii at Manoa * http://www.pbrc.hawaii.edu/bemf* } **************************************************************************** }
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It's a bit late but may I wish you a happy new year.
My personal experience is that the biggest problem with CD writing is the possibility of corrupting the disk and not noticing (e.g. buffer under runs). This can at the least result in wasted time and frustration and at worst the actual loss of data if not properly backed up elsewhere. I haven't seen this mentioned so I thought I would bring up the subject of 'Burn proof' CD writers which have appeared in the last 6-12 months. They apparently have built in hardware/software which should mean that you can now use CDs as super floppies and not have to worry about turning off conflicting software before writing large chunks of data to CD. The magazine reviews have raved about this stating that you could play 'Quake' or access the internet and still write to a CD without error. Has anyone had any experience of these new drives?
Archival quality of CDs, ZIPs and magneto opticals has been discussed many times before and the usual conclusion is that the technology will be defunct before good quality discs, stored properly will be significantly corrupted. My money has to stay with CDs as a cheap, reliable and 'likely-to-be-around-in-a-decade' technology (e.g. all modern DVD drives still read CDs). CD/DVD technologies still have a long way to go in terms of data density and so multi-format reading machines would seem more likely than with magnetic media ... unless you know better. I'm sure that I read of recent developments in dyes/pigments (maybe it was Kodak - I don't know) that should greatly reduce writeable CDs deterioration in light. One thing's for certain if I want to distribute images to students, researchers or other users there is only one universal technology (some new PCs don't even have a floppy drive now).
Another thread was discussing e.m. film scanners and I think I should mention the Epson Perfection 1200P which is a USB scanner that can be used with A4 prints or 5x4 inch negatives. It has a true resolution of 1200dpi and an optical density range of 3.2 and costs a little over 200 UK pounds. Much of our work with undergraduates and researchers has been done at 600dpi (which should easily allow an equivalent of 3x print enlargement) and dare-I-say-it JPEG formats (set at lowest compression to retain most detail). The film is, after all, our archive and the digital images are at present for cataloguing, rapid retrieval and project write ups - the students love it if only because they don't spend hours in the darkroom. I am not suggesting that this particular scanner will suit all users because it has a narrower OD range than some, but is an excellent low cost way of trying the technology out while it is still maturing. The biggest problem is that there was no film holder for our format but cardboard and sticky tape have solved that problem, temporarily. Also if you opt for the USB version then you really need Windows 98 on a PC (95 - including the the second version, NT etc. may all have problems).
I have no commercial interest in any of the above technologies unless they make my work or research any easier - in a year or two I may be in a better position to judge that, objectively.
Malcolm Haswell e.m. unit University of Sunderland UK
ERIC 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 } -----------------------------------------------------------------------. } } On the HP CD Writer there are two programs for writing to a CD.. Out here } we use the CD-R one time write to the disc. } } There is the HP program for writing a CD which does not have a way to } verify the CD was written. There is also another program that comes with } the CD writer from HP that performs a write speed test on the disc then } writes to the disc and then it verifies the disc... the program is called } MY CD on the HP CD writers....
I agree, but I don't blame the film makers. They are part of the majority of the public who (sometimes proudly) proclaim to have no/little knowledge of science. It seems to be quite common to use bugs, germs, viruses, bacilli and bacteria as interchangeable terms. This can be extremely misleading when a national news reporter warns of the latest outbreak of the meningitis 'virus' when he almost certainly meant the bacterial form.
There has been more than one occasion where I have seen a TEM instrument with a superb SEM image portrayed on film or TV (yes I know about TEM/SEM/STEMs - but it wasn't) presumably because the TEM looks impressive and so do SEM pictures. I also saw the Bladerunner SEM and another technology it had was a voice activated TV with high resolution scanner and printer. It seemed well out of reach of the average household at the time and although I haven't seen this on a TV this month all of that technology is common on your average home PC now - maybe the next Intel (QX4) microscope will be a toy SEM connected to your TV.
Malcolm Haswell e.m. unit University of Sunderland UK
} ------------------------------------------------------------------------ } 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 } -----------------------------------------------------------------------. } } Around 20 years ago, I saw a movie about killer bats in which, after looking } at a slide with what looked like a Tasco microscope, the scientist exclaimed } "It's just as I feared - the rabies bacillus!". To add insult to injury there } followed a view through the microscope where, if I recall correctly, a } paramecium was swimming. } } Paul
At 07:22 PM 1/8/01 -0800, Gary Gaugler wrote: } They are all dye-based. What is silver or gold is the coating } on the top of the media. It ca readily be flaked off.
No, supposedly the gold ones are actually made of gold the metal, and the "silver" ones are aluminum. The Al will oxidize over time if scratched, the Au won't.
The story says that if you scratch a disc deep enough to expose the metal, it could degrade the data over time. I don't put a lot of stock in this worry, though. After all, it wouldn't take much more of a scratch to wipe out a section of gold, too, and there's a big difference in damage between a radial and a concentric scratch on any media.
Thanks for coming up with the reference. I just KNEW it was it my Reference Manager database (NOT). So, for several days now I have been trying to figure out if I ever referenced it in a paper, or in notes or methods/techniques/procedures.... Now I can sleep at night again :)
Roger Moretz, Ph.D. Dept of Toxicology Boehringer Ingelheim Pharmaceuticals, Inc.
On Mon, 08 Jan 2001 12:45:29 -0800, Michael Nesson 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 } -----------------------------------------------------------------------. } } } } } Gordon Couger wrote: } } } } } Could someone post the reference for the article for making glass knives } } by hand? } } Here's the original reference, which includes a bit of the history of Ralph } knives (in honor of the late Dr. Paul Ralph): } Stain Technology 51(2): 71-97. [1976]. Bennet et al. } Science and art in preparing tissues embedded in plastic for } light microscopy, } with special reference to glycol methacrylate, glass knives and } simple stains. } } Good luck. } Mike Nesson } _______________________________________________________________________ } Michael Nesson, Ph.D. Department of Biochemistry & Biophysics } 2011 Ag&LS, Oregon State University, Corvallis, OR 97331-7305 } (541)737-5245 FAX:(541)737-0481 nessonm-at-ucs.orst.edu } } }
_______________________________________________________ Send a cool gift with your E-Card http://www.bluemountain.com/giftcenter/
Our customers have enjoyed success with the Agfa "Duoscan" line of scanners. Fitting in your price range would be the Duoscan Hi-D. The Hi-D has a Dmax of 3.8 (hence the name Hi-D), 1000x2000 hardware resolution, apochromatic optics, excellent software for both Mac and Windows, color management software, and a SCSI interface. The Hi-D sells for under $2600. Coming soon will be the Arcus 1200, which also has glassless film scanning, 1200x2400 hardware resolution with a SCSI interface. The Arcus 1200 will be approximately $800-850 when available. The Agfa T2500 is a similar design, with 2500x2500 hardware resolution and 3.4 Dmax. The T2500 does not fall in this price range, selling for under $4300. It is a phenomenal scanner for TEM. There is currently a $350 rebate on the T2500. All of these scanners share the Agfa Fotolook sofware driver for Mac and Windows. Unlike most "flatbed" scanners which place films on a glass bed for scanning, the Duoscan line utilizes a glassless holder similar to a negative carrier in an enlarger. There is no glass between the film and the CCD. This eliminates Newton Rings and other issues associated with scanning through glass.
Microtek International shares some hardware specs with the Agfa Duoscan line in their Artixscan series. The Artixscan 1100 would be the "sister" model to the Duoscan Hi-D with 1000x2000 optical resolution, 3.9 Dmax, SCSI interface,etc. Price is under $1750. The Artixscan 2500 is similar to the Duoscan T2500- 2500x2500 optical res, SCSI interface, etc. Price under $4000.
See Microtek at http://www.microtekusa.com/list.zhtml?cid=2 Agfa DuoScan HI-D at http://www.agfahome.com/product/CatProd_DisplayPublic.html?id=4290 Agfa DuoScan T2500 at http://www.agfahome.com/product/CatProd_DisplayPublic.html?id=3115 Agfa Arcus 1200 at http://www.agfahome.com/product/CatProd_DisplayPublic.html?id=6130
I will be happy to provide literature, information or answer any questions. Please contact me directly by phone or email.
Sincerely,
George
George Laing National Graphic Supply v:(800) 223-7130 X3109 f:(800) 832-2205 email: scisales-at-ngscorp.com
Hello, I was wondering if any one might know where I could get some cryostat tissue mounting stubs. I am looking for the 'T' type looking stubs that fit into a ball joint so the stub position can be adjusted in the cryostat chuck. The ones I have used were made of copper and the pin diameter was1/8" with a locking screw in the shaft of the ball joint. Thanks for any leads. Sincerely, Jonathan
Jonathan Wilson (Ph.D.) Centro Interdisciplinar de Investigação Marinha e Ambiental (CIIMAR) Universidade do Porto Rua do Campo Alegre 823 4150-180 Porto, Portugal tel 351 22 606 0421 fax351 22 606 0423 e-mail: wilson_jm-at-cimar.org mop01258-at-mail.telepac.pt
Many years ago (at least 6!) when we had an early Pinnacle Micro CD writer I got into the habit of checking my CD's by copying them back to the hard drive. If they would copy without generating an error then they were OK (an even better way was to do the copy on another CD drive). One fairly often found one that was bad.
Today, using a more modern drive and faster computer I still do the same thing (my software doesn't have a verify option), but I rarely find a bad disk. However, it doesn't take much of my time, and I always think better safe than sorry when it comes to an archive!
I need to get some parts for a RMC MX-600XL ultramicrotome.. I know RMC was sold to another company from Ventana.. How do I or who do I contact about some parts??
Eric A. Rosen UCLA Medical Center Dept. Pathology and Lab Medicine Los Angeles, CA 90095
In the context of recent queries, I just thought I'd post Nikon's most recent announcement ... see: http://www.klt.co.jp/Nikon/Press_Release/ls-8000.html
cheerios, shAf :o)
{} /\ {\/} /\ {\/} /\ {\/} /\ cogito, ergo zZOooOM /\ {\/} /\ {\/} /\ {\/} /\ {} Michael Shaffer, R.A. - mshaf-at-darkwing.uoregon.edu Geological Science's Electron Probe Facility - University of Oregon http://epmalab.uoregon.edu/
In the context of recent queries, I just thought I'd post Nikon's most recent announcement ... see: http://www.klt.co.jp/Nikon/Press_Release/ls-8000.html
cheerios, shAf :o)
{} /\ {\/} /\ {\/} /\ {\/} /\ cogito, ergo zZOooOM /\ {\/} /\ {\/} /\ {\/} /\ {} Michael Shaffer, R.A. - mshaf-at-darkwing.uoregon.edu Geological Science's Electron Probe Facility - University of Oregon http://epmalab.uoregon.edu/
In a message dated 01/09/2001 11:30:40 AM US Mountain Standard Time, biology-at-ucla.edu writes:
{ { I need to get some parts for a RMC MX-600XL ultramicrotome.. I know RMC was sold to another company from Ventana.. How do I or who do I contact about some parts??
Eric A. Rosen UCLA Medical Center Dept. Pathology and Lab Medicine Los Angeles, CA 90095
} }
Eric,
RMC is now a part of Boeckler Instruments in Tucson, Arizona. You can reach them at:
Boeckler Instruments, Inc. 4650 South Butterfield Drive Tucson, AZ 85714 Tel. 800-552-2262 Fax 520-745-0004
I have a Kevex EDS detector that was shipped via FEDEX with liquid nitrogen. FEDEX, in their infinite wisdom, managed to tilt the detector and drain the LN2 from the dewar. (Although the packing box and "tilt watch indicators" say "do not tilt', "this side up", etc.)
Upon inspecting the detector I have found that a plug on the side of the dewar has been removed and the detector is at atmosphere. I suspect that the LN2 froze the plug & "O" rings therby allowing air into the detector.
I am considering machining an adapter flange and repumping the detector. This is, of course, assuming that the detector window is entact.
Does anyone have experience with this? While pumping, I am considering pouring hot water into the dewar to outgass the system but I don't know if this is a good idea.
Hi - I am looking for a used lens regulator circuit board for a Philips TEM 201. The parts # is Lens Regulator 5322 695 14022 in the 1974 service manual -also called RB-U13. Is anyone junking a 201? The price from FEI/Philips is a bit beyond my budget! g
Hi - I am looking for a used lens regulator circuit board for a Philips TEM 201. The parts # is Lens Regulator 5322 695 14022 in the 1974 service manual -also called RB-U13. Is anyone junking a 201? g
Colleagues, Has anyone had any experience with generating energy filtered diffraction patterns (not CBED) with a Gatan GIF on a Philips CM? I would like some pointers on intensity issues and summation of images. Thanks in advance. Ciao for now, Ken
We are installing a new JEOLCO JSM 6700F Field Emission Scanning Electron Microscope. This is a new model and incorporates some novel technology. We are interested in communicating with others who are or will be working with this model. Please respond off-line and I will construct a mailing list to distribute questions, concerns and, of course, suggestions for operation and improvement.
James R. Coleman, Ph.D. Supervisor, Electron Microscopy Laboratories Boehringer-Ingelheim Pharmaceuticals Inc.
Richard asked if the exposure meter on the Nikion coolpix 900 digital camera was sensitive enough to control exposure in low light (immunofluorescent) conditions. We used the camera to take images of samples labeled with moderate intensely with FITC. We captured nice images in the "spot" automatic metering mode. With the camera mounted in one ocular, the camera chose to expose at F 3.1 and kept the shutter open one second. However, it was a bit difficult to use since the image did not appear on the display during focusing. There was not enough light for real time imaging. To insure a focused image, we needed focus in brightfield illumination, then go to EPI to collect the image. You could also use a monitor, but that would add significant cost to the system.
It may be useful to realize that the camera has the ability to be used in several automatic exposure settings (programmed, aperture priority, shutter priority) (wide field, narrow field, center spot) and in manual mode, where you can use a timed exposure from 1/1000 to 8 seconds, or longer (up to 60 seconds) by pushing the exposure once to open and again to close.
Feel free to phone with more questions,
Doug
---------------------- Douglas R. Keene Associate Investigator Shriners Hospital Research Facilities 3101 S.W. Sam Jackson Park Road Portland, Oregon 97201 phone: 503-221-3434 FAX: 503-412-6894 (9-5 PST) e-mail: DRK-at-shcc.org
It all depends. If there is no-one else who would pay to fix your detector, then you have nothing to lose by doing what you suggest (incl. the hot water). I do it relatively often, (but only to detectors that are seriously degraded or not functioning at all), and it works, but I've never had a crystal return to tip-top premium performance after this treatment. (In fact, only today I deliberately vented a detector and re-pumped it, but that is a long, and different, story). BTW, you only need to achieve a quite modest vacuum during the pump - the molecular sieve will take care of a lot of gas when it cools! Having said that, I have usually rigged up a piece of vacuum hose from the pumping adapter to a port I had added to an old evaporater, and pumped down to the 10^-5 - 10^-4 range. I have a pumping adapter with a US thread for the plug - perhaps it will work on your Kevex detector (in fact, it came from Kevex 20 years ago). If you want to borrow it, let me have your FedEx or other shipping account number, and shipping details, and I'll send it off.
On the other hand, if the shipper, or FEDEX, can be persuaded to pay to have the detector refurbished, it will probably work better in the end, and a do-it-yourself attempt beforehand may make your claim more difficult!
Good luck!
Tony
Tony.
At 02:07 PM 1/9/2001 -0800, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
I suppose, if plastic film or plastic sections (biological samples) are relatively stable under the beam, it may mean (may not) that temperature is not so high. In my hands, overheating of the plastic film in air over +150oC will destroy the film. I assume, something like that would happens in the microscope if the beam generate such amount of heat (plastic film itself has a low thermal conductivity, I believe). Another scenario: unelastic scattered electrons may transfer kinetic energy (not necessary it will immediately transferred into the heat) to the sample/film. This excess of energy may heat the sample but may force molecules/atoms to migrate for instance. Heavy atoms should affected more. I do remember, 20 or so years ago people shout films under TEM, how Pt or Au atoms may move under the beam. They (atoms) tend to form big clusters under the beam. This is explanation (to me), why the resolution of Pt or Au shadowed samples is so bad. Pt-C shadowing succeeded because carbon protect Pt from migration and forming big clusters. In general, I do agree: "it depends"...
Sergey
At 09:39 AM 1/9/01 +0000, 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
I did a few detector treatments and I agree with Tony's comments. One addition: Obtain a fairly good vacuum before pouring boiling water (couple of liters) into the dewar. The heat causes a dramatic drop in vacuum due to outgasing of the molecular sieve. I would terminate pumping a couple of hours after the hot water was added. Obviously is nice to have a clean vacuum system available as backstreaming oil vapour would rather defeat the purpose. Cheers Jim Darley ProSciTech Microscopy PLUS PO Box 111, Thuringowa QLD 4817 Australia Ph +61 7 4774 0370 Fax:+61 7 4789 2313 service-at-proscitech.com Great microscopy catalogue, 500 Links, MSDS, User Notes ABN: 99 724 136 560 www.proscitech.com
On Wednesday, January 10, 2001 1:37 PM, Tony Garratt-Reed [SMTP:tonygr-at-mit.edu] wrote: } } } Earl- } } It all depends. If there is no-one else who would pay to fix your } detector, then you have nothing to lose by doing what you suggest (incl. } the hot water). I do it relatively often, (but only to detectors that are } seriously degraded or not functioning at all), and it works, but I've never } had a crystal return to tip-top premium performance after this treatment. } (In fact, only today I deliberately vented a detector and re-pumped it, but } that is a long, and different, story). BTW, you only need to achieve a } quite modest vacuum during the pump - the molecular sieve will take care of } a lot of gas when it cools! Having said that, I have usually rigged up a } piece of vacuum hose from the pumping adapter to a port I had added to an } old evaporater, and pumped down to the 10^-5 - 10^-4 range. I have a } pumping adapter with a US thread for the plug - perhaps it will work on } your Kevex detector (in fact, it came from Kevex 20 years ago). If you } want to borrow it, let me have your FedEx or other shipping account number, } and shipping details, and I'll send it off. } } On the other hand, if the shipper, or FEDEX, can be persuaded to pay to } have the detector refurbished, it will probably work better in the end, and } a do-it-yourself attempt beforehand may make your claim more difficult! } } Good luck! } } Tony } } Tony. } } } At 02:07 PM 1/9/2001 -0800, 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 } } -----------------------------------------------------------------------. } } } } } } Hi all, } } } } I have a Kevex EDS detector that was shipped via FEDEX with liquid nitrogen. } } FEDEX, in their infinite wisdom, managed to tilt the detector and drain the } } LN2 from the dewar. } } (Although the packing box and "tilt watch indicators" say "do not tilt', } } "this side up", etc.) } } } } Upon inspecting the detector I have found that a plug on the side of the } } dewar has been removed and the detector is at atmosphere. I suspect that the } } LN2 froze the plug & "O" rings therby allowing air into the detector. } } } } I am considering machining an adapter flange and repumping the detector. } } This is, of course, assuming that the detector window is entact. } } } } Does anyone have experience with this? While pumping, I am considering } } pouring hot water into the dewar to outgass the system but I don't know if } } this is a good idea. } } } } Thank You, } } } } Earl Weltmer } } } *********************************************** } Anthony J. Garratt-Reed, M.A., D.Phil. } Principal Research Scientist } Room 13-1027 } Massachusetts Institute of Technology } 77 Massachusetts Avenue } Cambridge, MA 02137-4307 } } Tel: (617) 253-4622 } Fax: (617) 258-6478 } ***********************************************
If you have a problem locating the original suppliers of these object holders, I should be able to make them for you, please fax me a sketch will measurement and I will reply with a price.
Best Regards
Alan Bright
Bright Instrument Co.Ltd. St Margaret's Way Huntingdon Cambridgeshire PE29 6EU England
Tel No:+44 (0)1480 454528 Fax No:+44 (0)1480 456031 Email: AlanBright-at-brightinstruments.com Web Site: www.brightinstruments.com
-----Original Message----- } From: Jonathan Wilson [mailto:wilson_jm-at-cimar.org] Sent: 10 January 2001 00:31 To: Microscopy
Hello, I was wondering if any one might know where I could get some cryostat tissue mounting stubs. I am looking for the 'T' type looking stubs that fit into a ball joint so the stub position can be adjusted in the cryostat chuck. The ones I have used were made of copper and the pin diameter was1/8" with a locking screw in the shaft of the ball joint. Thanks for any leads. Sincerely, Jonathan
Jonathan Wilson (Ph.D.) Centro Interdisciplinar de Investigação Marinha e Ambiental (CIIMAR) Universidade do Porto Rua do Campo Alegre 823 4150-180 Porto, Portugal tel 351 22 606 0421 fax351 22 606 0423 e-mail: wilson_jm-at-cimar.org mop01258-at-mail.telepac.pt
For about 15 years, I ran a Kevex "extra" detector. This was a windowless type and over time (I did a lot of light element work) the crystal would ice over. The Etec was turbo pumped, but between specimen out gassing and the methane from the WDS, icing over time could not be avoided. I warmed and pumped a number of times using warm/hot water. A small amount of degradation occurred, but it did help overall. I later went to a hot air gun and a tube to direct the air to the bottom of the dewar. By doing this, I did not have to worry about drying the dewar.
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Several folks have asked about chillers and evaporators lately.
We have a Denton DV-515 vacuum evaporator which has been replaced by an automated DV-502A. The DV-515 was originally from a government lab so it has been well maintained and cared for. We had used it mainly as a back up for our DV-502A. We use the carbon rod arc to produce TEM support films and general carbon coating of samples on MCE & PC filters during TEM specimen prep and to put carbon coatings on SEM samples.
If you are interested, we would like 2500. reply to:
All, The preliminary information I have is that the Coolscan 8000 ED will sell for approximately $4000 US. We will carry it when it becomes available, currently listed as June. I hope to see it in early February. Quick specs.. 4000dpi optical resolution IEEE1394 "Firewire" Interface- not SCSI 4.2 dynamic range 48bit images Multi Sample Scanning
Info is also at http://64.77.39.20/usa_product/product.jsp?cat=7&grp=703&productNr=9246
I'll pass along more info as it becomes available.
George
George Laing National Graphic Supply v:(800) 223-7130 X3109 f:(800) 832-2205 email: scisales-at-ngscorp.com } } This looked pretty interesting. Have you heard a ballpark price? } } } } } In the context of recent queries, I just thought I'd } } post Nikon's most recent announcement ... see: } } http://www.klt.co.jp/Nikon/Press_Release/ls-8000.html } }
I called Nikon yesterday (1/9/2001) to ask about the Coolscan 8000 ED. They told me it would cost $3000 (U.S.) and is scheduled to be released in April.
Question: I need to view calcium carbonate crystals with a transmission electron microscope for a research project. I also need to record the images. All I've managed to do so far is order thin carbon grids. I have been asked to write a plan for my experiment but I have no clue how to prepare crystals in solution for magnification or what tools to use. Please give me some direction. My professors say I should figure everything out myself - "It will be a good learning experience."
Dear Jane, The most difficult aspect of this is likely to be getting sufficiently small crystals dispersed over the grid surface so that you can see the individual crystals. You do not say whether you need detail within the crystals or whether just seeing silhouettes is sufficient. If the latter, then just evaporate the solvent rapidly from a dilute CaCO3 solution placed on the grid. This should leave small crystals dispersed over the grid. If you can't evaporate on the grid, you will have to prepare the small crystals and transfer them either by suspending them in a volatile liquid which doesn't dissolve CaCO3 or by wafting them into the air and collecting them on the grid. If you need detail within the crystals, they must be very thin--no more than ~10 nm (depending on the EM voltage), so you will have to find a way to get them this thin, and, if possible, much wider than they are thin--a platy habit. Good luck. Yours,
Bill Tivol Wadsworth Center Albany NY (518) 473-7399 WFT02-at-health.state.ny.us
Can anyone answer this question . Remember Ask-A-Microscopist is a forum that is used by NON-MICROSCOPISTS looking for help so keep try to your technical details at the right level.
Email: us004118-at-mindspring.com Name: Leonard Lessin, FBPA
School: (Retired Science & Medical Photographer)
State: NY
Zip: 10012
Question: I am enjoying doing photomicrographs of crystal preperations in polarized light.However I have insuffient knowledge of chemistry to choose solvents without a long series of trial and error efforts.Can you give me a rationale and/or a reference to go about this in a more productive manner?
Dear Leonard, There are several requirements for a suitable solvent: 1) it must, of course, disolve the material you want to examine, 2) it must evaporate to produce crystals in a habit suitable for your work (not too small, transparent, etc.), and 3) it should not be too toxic even though you may have a fume hood available. The key to 1) is "like disolves like". If you have an ionic salt or a polar solute such as sucrose, water would be a good choice, if you have an aromatic compound, such as naphthalene, an aromatic would work (I hesitate to reccommend benzene, even though it gives nice crystals, because of its toxicity; I would try toluene.), and if you have a lipid, like cholesterol, I'd use a non-polar aliphatic solvent such as hexane. For 2) it is important to have a suitable rate of evaporation, so in the last case, hexane might evaporate too fast, so I would go to a longer-chain hydrocarbon, e.g., decane. The Handbook of Chemistry and Physics lists many compounds, both organic and inorganic, and some solvents for each; I'd use that as a first reference. I hope this will reduce the problem from a long series of trial-and-error efforts to a short one, but you can still expect some problems. The preparation of suitable crystals is most often the most difficult part of these studies. Good luck. Yours,
Bill Tivol Wadsworth Center Albany NY (518) 473-7399 WFT02-at-health.state.ny.us
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I was forced to dismantle my Opti-quip fluorescence bulb housing the other day for an unrelated problem. The 75W xenon bulb only has 200 hrs of use so I would have expected it to have another 200 hrs of life based on what the supplier told me. But I noticed that at one of the ends, at the junction between the metal cap and the glass bulb, there was a buildup of a hard, white substance on the outside of the glass. Does any one know what caused this and if it is safe to re-install the bulb? TIA, tom
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Thermo NORAN, the makers of the finest instrumentation for elemental analysis is seeking both a Microanalysis and an XRF Applications/Product Specialist. This position will be responsible for the ensuring the success of the applications/products targeted at analytical instrument markets, including materials characterization and materials development markets. Will perform demonstrations and provide other pre-sale support as required at major trade shows, technical conferences and other meetings. Will analyze customer samples and prepare reports for prospective customers. Worldwide travel may be required to perform demonstrations and presentations. Travel may include trips greater in duration than one week. Must be degreed in a physical or life science, have excellent written and oral communication skills. Knowledge of electron microscope and/or x-ray microanalysis with experience in materials characterization. Interested candidates should send, e-mail or fax resumes to:
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I'm writing up a wish list for our EM lab, and it includes (gasp) light microscopes. My question is - how do I go about evaluating and choosing a digital camera for light microscopes? It would be for both compound and dissecting microscopes, should be color, decent resolution, not necessarily low light nor real-time video, but capable of good images for image analysis on sections. We are getting a confocal, so fluorescence imaging would be done there rather than with the proposed 'scope and camera.
What do I need to look for, and what price ranges are we talking about?
Mahalo, Tina
http://www.pbrc.hawaii.edu/bemf/microangela **************************************************************************** * Tina (Weatherby) Carvalho * tina-at-pbrc.hawaii.edu * * Biological Electron Microscope Facility * (808) 956-6251 * * University of Hawaii at Manoa * http://www.pbrc.hawaii.edu/bemf* ****************************************************************************
Does anyone know how to mount large (100um+) diatoms for LM or SEM? The little ones are OK, they stick to most any stub, but these big guys like to fall off.
Anyone know how arranged diatom slides are/were made? I checked WWW but no specifics on techniques. Something like these methods would work for us.
Thanks
Jonathan Krupp Microscopy & Imaging Lab University of California Santa Cruz, CA 95064 (831) 459-2477 jmkrupp-at-cats.ucsc.edu
Richard asked if the exposure meter on the Nikion coolpix 900 digital camera was sensitive enough to control exposure in low light (immunofluorescent) conditions. We used the camera to take images of samples labeled with moderate intensely with FITC. We captured nice images in the "spot" automatic metering mode. With the camera mounted in one ocular, the camera chose to expose at F 3.1 and kept the shutter open one second. However, it was a bit difficult to use since the image did not appear on the display during focusing. There was not enough light for real time imaging. To insure a focused image, we needed focus in brightfield illumination, then go to EPI to collect the image. You could also use a monitor, but that would add significant cost to the system.
It may be useful to realize that the camera has the ability to be used in several automatic exposure settings (programmed, aperture priority, shutter priority) (wide field, narrow field, center spot) and in manual mode, where you can use a timed exposure from 1/1000 to 8 seconds, or longer (up to 60 seconds) by pushing the exposure once to open and again to close.
Feel free to phone with more questions,
Doug
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Listers My company's safety folks are bent on making us wear Kevlar gloves while razor trimming samples for ultramicrotomy - I'm talking about the final trimming done using a trimming stand on the microtome. As you might know, this is fine work - wearing gloves is a handicap. My questions: 1. Does anyone out there actually wear gloves? - if so then can you recommend a glove? 2. Are there other ways to make this task look less dangerous to the safety police? (short of purchasing a trimming machine)
Thanks!
Dave Calvert Eastman Chemical Company Building 150B Lincoln Street (packages) P.O. Box 1972 (US Mail) Kingsport, Tennessee 37662-1972 (423) 229-4943 (423) 229-4558 fax
} My company's safety folks are bent on making us wear Kevlar gloves while } razor trimming samples for ultramicrotomy - I'm talking about the final } trimming done using a trimming stand on the microtome. As you might know, } this is fine work - wearing gloves is a handicap. } My questions: } 1. Does anyone out there actually wear gloves? - if so then can you } recommend a glove? } 2. Are there other ways to make this task look less dangerous to the } safety police? (short of purchasing a trimming machine)
When I train people to trim blocks, I always point to the Band-Aids first, then to the razor blades! This gets a laugh, but drives home the point. Then I suggest that they put the bandages on FIRST before trimming, which also gets a laugh, but significant number of people decide to do so! Therefore, I suggest something like finger cots or other wrap-around solutions that leave some dexterity while protecting the last joints of the fingers.
Aloha, Tina
http://www.pbrc.hawaii.edu/bemf/microangela
**************************************************************************** * Tina (Weatherby) Carvalho * tina-at-pbrc.hawaii.edu * * Biological Electron Microscope Facility * (808) 956-6251 * * University of Hawaii at Manoa * http://www.pbrc.hawaii.edu/bemf* ****************************************************************************
Jonathan Krupp wrote: ============================================================== Does anyone know how to mount large (100um+) diatoms for LM or SEM? The little ones are OK, they stick to most any stub, but these big guys like to fall off.
Anyone know how arranged diatom slides are/were made? I checked WWW but no specifics on techniques. Something like these methods would work for us. ============================================================== Consider these two options:
a) Tacky Dot™ Slides, see URL http://www.2spi.com/new/tacky.html and b) Double sided conductive discs, sheets or tape http://www.2spi.com/catalog/spec_prep/cond_adhes.html
The Tacky Dot Slides have good adhesion and the diatoms should be held in place without problems. The double sided conductive sheets, discs, and tape should work as well, but if you are using material that has aged past its "expiration date", the surface tends to lose its "tac" and indeed might not hold the "big guys". Of course, only the Tacky Dot Slides will result in the diatoms being arranged in orthogonal arrays for convenient analysis.
Disclaimer: SPI Supplies is the exclusive worldwide licensee for the manufacturing and distribution of Tacky Dot Slides for applications in microscopy and microanalysis.
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 ############################ ==================================================
Klaus Kemp at http://www.diatoms.co.uk/index.html makes stunning arrangments of diatoms and seems willing to share his knowledge.
Gordon Gordon Couger gcouger-at-couger.com Stillwater, OK www.couger.com/gcouger
} From: "Jon Krupp" {jmkrupp-at-cats.ucsc.edu}
} } Hi: } } Does anyone know how to mount large (100um+) diatoms for LM or SEM? The } little ones are OK, they stick to most any stub, but these big guys like to } fall off. } } Anyone know how arranged diatom slides are/were made? I checked WWW but no } specifics on techniques. Something like these methods would work for us. } } Thanks } } Jonathan Krupp } Microscopy & Imaging Lab } University of California } Santa Cruz, CA 95064 } (831) 459-2477 } jmkrupp-at-cats.ucsc.edu } } }
Never cut myself in over quarter a century of trimming. Any accidental cuts would be minor since little force is exerted during final trimming. Some force is required during rough trimming and when cutting PE moulds off blocks - without a press. For these operations, just think where a slipped razor blade may go - and that is were the fingers don't. Surprizingly hardly anybody in my labs ever cut a finger, because they were taught the obvious. I think its also obvious, that unless those Kevlar gloves are rather thick (no analogy to the safety police) they would not prevent cuts. They should have recommended those stainless steel chain linked butcher's gloves. That could be a saleable idea! Cheers Jim Darley ProSciTech Microscopy PLUS PO Box 111, Thuringowa QLD 4817 Australia Ph +61 7 4774 0370 Fax:+61 7 4789 2313 service-at-proscitech.com Great microscopy catalogue, 500 Links, MSDS, User Notes ABN: 99 724 136 560 www.proscitech.com
On Thursday, January 11, 2001 10:03 AM, Calvert, Dave [SMTP:calvert-at-eastman.com] wrote: } } } } Listers } My company's safety folks are bent on making us wear Kevlar gloves while } razor trimming samples for ultramicrotomy - I'm talking about the final } trimming done using a trimming stand on the microtome. As you might know, } this is fine work - wearing gloves is a handicap. } My questions: } 1. Does anyone out there actually wear gloves? - if so then can you } recommend a glove? } 2. Are there other ways to make this task look less dangerous to the } safety police? (short of purchasing a trimming machine) } } Thanks! } } Dave Calvert } Eastman Chemical Company } Building 150B Lincoln Street (packages) } P.O. Box 1972 (US Mail) } Kingsport, Tennessee 37662-1972 } (423) 229-4943 } (423) 229-4558 fax } }
I have always worn latex gloves more for protection ( abrasion from tightening chucks, etc.) Using long single edge razors (Weck Extra Long Blades, EMS #71933-60) seems to give me more control of the blade and therefore less of a chance to knick one's fingers.
Becky Garrison Pathology Supervisor Shand Jacksonville Jacksonville, FL 32209 904-244-6237 -----Original Message----- } From: Calvert, Dave [mailto:calvert-at-eastman.com] Sent: Wednesday, January 10, 2001 7:03 PM To: Microscopy-at-sparc5.microscopy.com
Listers My company's safety folks are bent on making us wear Kevlar gloves while razor trimming samples for ultramicrotomy - I'm talking about the final trimming done using a trimming stand on the microtome. As you might know, this is fine work - wearing gloves is a handicap. My questions: 1. Does anyone out there actually wear gloves? - if so then can you recommend a glove? 2. Are there other ways to make this task look less dangerous to the safety police? (short of purchasing a trimming machine)
Thanks!
Dave Calvert Eastman Chemical Company Building 150B Lincoln Street (packages) P.O. Box 1972 (US Mail) Kingsport, Tennessee 37662-1972 (423) 229-4943 (423) 229-4558 fax
I have used LKB (now Reichert-Jung or whatever) microtomes and it has always been possible to trim specimen blocks with glass knives on the microtome, itself. With a bit of practice you can both trim and cut within about 30 minutes per block so I don't think that it's particularly time consuming. The added bonuses are that blocks will always have smooth facets and students get some good hands-on training with microtome, binoculars and knives before actually cutting thin sections.
Once you get into the technique there are other rewards such as the ability to 'face' or smooth block fronts for best quality sections on difficult specimens, mesa trimming, combining trimming of blocks and light microscopy surveys etc. The only requirements are that your specimen must be embedded near to the surface of the resin for easy trimming and that you don't damage the microtome mechanism.
The basic technique is fairly intuitive you just need practice: trim the front of the block until you reach the specimen (1-5 um cuts on manual feed should be OK) rotate the knife stage by +10 to +40 deg (angle is optional and can be varied for each side) and trim until you reach the desired edge in your block rotate knife stage to the other side (i.e. -10 to -40deg) and again trim until you have a long thin block face rotate block in specimen holder by 90deg and repeat for the other two edges Finally I may carefully trim or 'face' the front of the block for best results If you want to produce mesas then don't rotate the knife - just use it to trim a few microns around each side of the area to stand 'proud' as a mesa. If the the block is difficult and blunts the knife you may need to use a second knife, although this is not common Smoothest trimming results from thinnest cuts at slowest speeds, so always make the last couple of cuts on each edge about 1um or less.
If you're uncertain about the ability of your ultramicrotome to trim in this fashion, I'm sure the manufacturer or someone on the list should be able to help. If I do ever trim with a blade I use single edged razors and cut away from myself on an uncluttered work area, but this may only happen once or twice a year often when I'm demonstrating the method to students.
I'm sure that this has been mentioned on the list quite some time back but please contact me directly if you have any further questions although there must be lots of labs that have experience of this technique.
DISCLAIMER I have no commercial interest in LKB or Reichert, they just happen to be the instruments that I have grown up with.
Good luck
Malcolm
Malcolm Haswell e.m. unit University of Sunderland UK
Tina Carvalho 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 } -----------------------------------------------------------------------. } } } My company's safety folks are bent on making us wear Kevlar gloves while } } razor trimming samples for ultramicrotomy - I'm talking about the final } } trimming done using a trimming stand on the microtome. As you might know, } } this is fine work - wearing gloves is a handicap. } } My questions: } } 1. Does anyone out there actually wear gloves? - if so then can you } } recommend a glove? } } 2. Are there other ways to make this task look less dangerous to the } } safety police? (short of purchasing a trimming machine) } } When I train people to trim blocks, I always point to the Band-Aids first, } then to the razor blades! This gets a laugh, but drives home the } point. Then I suggest that they put the bandages on FIRST before trimming, } which also gets a laugh, but significant number of people decide to do } so! Therefore, I suggest something like finger cots or other wrap-around } solutions that leave some dexterity while protecting the last joints of } the fingers. } } Aloha, } Tina } } http://www.pbrc.hawaii.edu/bemf/microangela } } **************************************************************************** } * Tina (Weatherby) Carvalho * tina-at-pbrc.hawaii.edu * } * Biological Electron Microscope Facility * (808) 956-6251 * } * University of Hawaii at Manoa * http://www.pbrc.hawaii.edu/bemf* } ****************************************************************************
I am trying to find a way of looking at a cross section of a printed ink approx 10um thick on a PVC substrate. I am trying to measure the porosity of the ink so I guess some image analysis will be used. It is mainly a method of preparing the samples that has me a bit stumped. I have tried freeze fracturing and embedding the samples in resin then polising the surface. Neither are satisfactory. The microscopy techniques I have available are SEM and LM. Can anyone help?
Largish diatoms, like most other microfossils bigger than, say, 50 microns or so in diameter or length, can usually be handled under a binocular microscope with a very fine (00 or 000) artists' paintbrush. Just wet the brush with water (distilled, if it's going to matter) and touch the bug with it. It'll stick to the brush long enough for you to place it on a stub. When I'm looking at microfossils in the SEM, I can usually get them to stick to double-sided tape on a stub just by "dabbing" them on with the point of the brush. Orienting them can be a bit tricky, but you'll improve with practice. One problem with double-sided tape, though, is that once stuck on, a lot of the more delicate microfossils such as diatoms will break before they'll come loose. So you don't want to handle type specimens this way.... Another good way to stick such bugs down includes a little bit of Gum Tragacanth. An old micropaleontologists' standby, this stuff is available as a powder, which you mix with a little water to make a paste. You can glue individual bugs down with this, using your fine paint brush. It dries in a few seconds - and if you want to move/remove the bug later, just wet your brush and touch the bug. The gum redissolves and the specimen comes free. Unsightly gum residues on the bug will come off with a bit more application of your wet brush. Once mixed up and kept in a sealed little vial, the gum mixture should keep for months or years. A drop or two of clove oil in it will inhibit any possible mould growth, if you're going to keep it around for a while. One guy I used to work with liked to use bits of old undeveloped 35mm film. Apparently you can get small items to stick to such film really well if the specimen is wet. I've never tried this myself, though. And, of course, there's lots of micropaleontology texts out there with chapters on handling techniques. After reading all this, you're probably sorry you got me started. Anyway, good luck with the diatoms - they're among nature's most photogenic micro-organisms.
Frank Thomas MicroAnalysis Facility Geological Survey of Canada (Atlantic) Bedford Institute of Oceanography Dartmouth, Nova Scotia Canada
----- Original Message ----- } From: "Jon Krupp" {jmkrupp-at-cats.ucsc.edu} To: {Microscopy-at-sparc5.microscopy.com} Sent: Wednesday, January 10, 2001 4:54 PM
Hi Folks,
Does anyone know of a stain to differentiate PMN's from Macrophages for light microscopy?
for a 7 Hr Minicourse in Cryomicroscopy and Microanalysis
at the Microscopy Technology Center of San Joaquin Delta College in Stockton, CA
Everyone is welcome. Come, enjoy, and RSVP. Happy New Year
Delta Microscopy Society, & Northern California Microscopy Society Joint Meeting
WHEN: Jan 17, 18, 2001; Wed. and Thur.
WHERE: San Joaquin Delta College, Microscopy Technology Center, Stockton, CA
Please email or fax RSVP. See form below.
7 Hr Minicourse in Low Temperature Microscopy and Microanalysis by Dr. Patrick Echlin, Director of Cambridge Analytical Microscopy and member of Multi-Imaging Centre, University of Cambridge, UK
Image Database (Asset Management System) for Multi-Platform, Multi-Instrument Microscopy Laboratory, Dr Judy A. Murphy, San Joaquin Delta College, Microscopy Technology Center
January 17, 2001: Wednesday 12:00 - 1:00 pm Registration, Holt 121 1:15 - 1:30 pm Welcome and Introduction, South Forum Building 1:30 - 2:30 pm Minicourse Lecture 1 : Chemical-physics of water and ice 2:45 - 3:30 pm Minicourse Lecture 2: Sample cooling 3:30 - 4:30 pm Tour of Microscopy Technology Center, Holt 121 including Demo of Image Database 4:30 - 5:30 pm Minicourse Lecture 3; Sectioning and Fracturing Discussion Social 5:30 - 6:30 pm, Budd Lounge Light Buffet 6;30 - 8pm, Budd Lounge 8:00 - 9:00 Image Database Lecture
January 18, 2001: Thursday 8:00 - 8:45 am Registration, 121 Holt 9:00 - 10:00 am Minicourse Lecture 4: Freeze drying, freeze substitution and low temperature embedding 10:15 - 11 am Minicourse Lecture 5: Low temperature microscopy Discussion 11:15 - 1:00 Lunch 1:15 - 2:15 pm Minicourse Lecture 6: Low temperature microanalysis 2:30 - 3:30 pm Minicourse Lecture 7 : Imaging, artefacts and beam damage. Discussion
Any building or room changes will be posted in Holt 121.
Activities are being sponsored by: Gatan Inc., Oxford Instruments, Hitachi, JEOL, FEI, Ted Pella Inc., EMS/Diatome, Anatech, Cressington, LEO, Advanced Computers and Networking, Delicato Winery, Paul De Georgio and others to be identified later.
Please RSVP so we know what room sizes we will need, # of handouts, and how much food.
Cost to Students: $0 Cost to Other Registrants $15 (to defray cost of activities, handouts, etc.)
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Please email or fax RSVP
email to: murphyjudy-at-mediaone.net
FAX to: 209/954-5600 This is a central fax, so put Judy Murphy, Microscopy on top of fax.
Any questions, call Judy Murphy (209/954-5284) or Pat Kysar (209/954-5246)
Checks can be made out to Delta Microscopy Society and sent to: Judy Murphy, San Joaquin Delta College, Microscopy Technology Center, 5151 Pacific Ave, Stockton, CA 95207
Directions to Microscopy Technology Center & Lodging Holt Center San Joaquin Delta College 5151 Pacific Avenue Stockton, CA 95207
1. Find Interstate 5 (I-5) on California map. It is a main North/South Interstate in California. 2. From I-5, exit on March Lane going East. Continue on March Lane 1.6 miles until you reach the traffic light at Pacific Ave. 3. At Pacific Ave.turn LEFT, and go 0.3 miles until you reach the traffic light for Delta College. 4. Turn LEFT at Delta College Entrance. The street is labeled Yoguts going East and Delta College going West. 5. As soon you turn into Delta College Entrance, bear LEFT on the Campus Drive (called Burke-Bradley in some places). 6. Continue around on Campus Drive until you reach Holt 1 Parking Lot. Turn RIGHT into Holt 1 Parking Lot. 7. As soon as you turn into Holt 1 Parking Lot, take a sharp RIGHT turn to enter Holt 2 Parking Lot. 8. Park as close to the front of the parking lot as possible, closest to the buildings. 9. Since this is the first week of Spring semester classes, no tickets are issued, so you do NOT need a parking permit. 10. As you walk towards the buildings, you should first enter Holt building. Go to Holt 121 which is the Microscopy Center. 11. Any questions, call Judy Murphy (209/954-5284) or Pat Kysar (209/954-5246)
Lodging Within 1.5 miles of San Joaquin Delta College Prices were quoted Dec. 20, 2000, but check when you make reservations. All listed lodging is close to March Lane exit off Interstate 5
Red Roof Inn, 2654 March Lane, Stockton, CA, Phone: 209/478-4300 Fax: 209/478-1872; Rates: Single - $59.99; Queen or 2 Double - $65.99; King - $71.99; Suite - $87 and up depending on number of people.
LaQuinta, 2710 W. March Lane, Stockton, CA, Phone: 209/952-7800, Fax: 209/472-0732; Rates: King-$75; 2 Double Beds-$69, Complimentary Breakfast AAA, AARP,Senior Citizen Discount Rates: King-$71.25; 2 Double beds-$65.55
Radisson Hotel, 2323 Grand Canal Blvd., Stockton, CA, Phone 209/957-9090 Fax: 209/473-0739; Rates: $79 - $99. Canal Blvd is one block off March Lane.
Courtyard by Marriott, 3252 W. March Lane, Stockton, CA, Phone 209/472-9700, Fax: 209/472-9722; Rate: $89-104 . Marriott Residence Inn, 3240 W. March Lane, Stockton, CA, Phone: 209/472-9800 Fax: 209/472-9888; Rates: Studio - $119; 1 Bedroom - $124. Complimentary Breakfast every day. Rooms have Kitchens equipped with Stove, refrigerators, pots & pans etc
It sounds like the safety folks may be overzealous in their attempts to protect you from embedding resins. Once polymerized, the resins are considerably safer than the monomers. Since the plastic is no longer liquid, latex gloves would be more appropriate (if the individual is not allergic to latex).
A bigger concern, I would think, when working with polymerized plastic is the possible allergic reaction due to inhalation of the plastic chips. I strongly recommend the use of a dust mask if you are using a grinder or other mechanical device to shape the blocks.
} My company's safety folks are bent on making us wear Kevlar gloves while } razor trimming samples for ultramicrotomy - I'm talking about the final } trimming done using a trimming stand on the microtome. As you might know, } this is fine work - wearing gloves is a handicap. } My questions: } 1. Does anyone out there actually wear gloves? - if so then can you } recommend a glove? } 2. Are there other ways to make this task look less dangerous to the } safety police? (short of purchasing a trimming machine) -- ############################################################## 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/departments/shops/cem.html ##############################################################
I have no experience in EDS detector pumping, but a little bit in vacuum technology.
What do you think about heating the Dewar before pumping ?
That's what I do with sorbtion (zeolite) pumps used to prepump UHV vessel (to have a dry pumping before starting turbo or ion pump). I put a heater around the pump -in our case it would be hot water (hot air ? hot oil ? which temperture can support the Dewar assembly ?)- let it warm over the night, and close the venting valve.
You could do something similar with the detector : warm it at air pressure for a few hours (it schould dry too the zeolite) and than pump down with turbo, but pre-pump with dry backing pump to prevent oil contamination, as Jim mentioned. Than pump down until the Dewar is cold, with a base pressure of something like 10E-5 Torr. And after that, cool it with nitrogen.
What do you think about that ?
Bye
J. Faerber IPCMS-GSI (Institut de Physique et Chimie des Matériaux de Strasbourg Groupe Surface et Interfaces) 23, rue de Loess 67037 Strasbourg CEDEX France
} } } } My company's safety folks are bent on making us wear Kevlar gloves while } } razor trimming samples for ultramicrotomy } } 2. Are there other ways to make this task look less dangerous to the } } safety police? (short of purchasing a trimming machine)
We routinely use a Dremel moto-tool (available at your local hardware store) with thin cutting wheels (i prefer the ones from Small Parts, Inc that have an abrasive on one side and a very thin metal backing on the other side). Working in the hood to avoid the dust, we can trim dozens of blocks rapidly. I advise holding the block in a pliers in case you slip with the dremel but it really is very easy once you get used to it. -- 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)
If someone in your lab has a Perrot Fabry spectrometer, you can use it to mesure film thickness between 2 and 100 nm. You évaporate your film on a glass slide (LM slide), than you put a fine scratch on the film, than you evaporate a opticaly opaque film of silver or aluminum. Than on the Perrot Fabry, with a monochromatic light, you can see and mesure the hights of the siver setp, which covers the the film to bee mesured. You must know the wavelength of your light. You schould find the way to calculate this in any optics book. You must do a serie of different thickness to draw a calibration curve. Its very sensitiv and cheep,... if you have the Perrot Fabry of course
An other way, opticaly too, is on a LM with a Nomarski Prism. I used it 15 years ago, but I do know the way to make the optical montage. I remember that there is a monochromatique light, the Nomarski prism, the polariser and analyser, but what kind of objectif ? The sample must be scratched and silver covered as with the Perrot Fabry...
Can someone tell me something about that ?
Thanks
J. Faerber IPCMS-GSI (Institut de Physique et Chimie des Matériaux de Strasbourg Groupe Surface et Interfaces) 23, rue de Loess 67037 Strasbourg CEDEX France
I had a quick look at the specification of the Coolscan 8000ED and it seems to be aimed at TEM users with about 6x9cm films - I quote the largest areas from the web page: (6 x 9) 63.5 x 88.0mm (10,000x13,176 pixels); (Elect Micro) 56.9 x 83.7mm (8,964x13,176 pixels); My e.m. film is 4 x 3 5/16 inches or 83 x 102 mm with an absolute minimum picture area (without data) of 69 x 92mm so it may be a problem for some e.m.
users.
I must admit it's a great specification though.
Malcolm Haswell e.m. unit University of Sunderland UK
George Laing 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 } -----------------------------------------------------------------------. } } All, } The preliminary information I have is that the Coolscan 8000 ED } will sell for approximately $4000 US. We will carry it when it becomes } available, currently listed as June. I hope to see it in early February. } Quick specs.. } 4000dpi optical resolution } IEEE1394 "Firewire" Interface- not SCSI } 4.2 dynamic range 48bit images } Multi Sample Scanning } } Info is also at } http://64.77.39.20/usa_product/product.jsp?cat=7&grp=703&productNr=9246 } } I'll pass along more info as it becomes available. } } George } } George Laing } National Graphic Supply } v:(800) 223-7130 X3109 } f:(800) 832-2205 } email: scisales-at-ngscorp.com } } } } This looked pretty interesting. Have you heard a ballpark price? } } } } } } } } In the context of recent queries, I just thought I'd } } } post Nikon's most recent announcement ... see: } } } http://www.klt.co.jp/Nikon/Press_Release/ls-8000.html } } } } } }
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Reply to: RE: Ultramicrotomy safety issues It is possible to perform all the trimming steps needed to get a good block by using glass knives. Not only is it safer for the operator it also produces blocks with smooth, regular edges which are great for serial sectioning. More details provided on command.
Paul Webster.
Paul Webster, Ph.D House Ear Institute 2100 West Third Street Los Angeles, CA 90057 phone:213 273 8026 fax: 213 413 6739 e-mail: pwebster-at-hei.org http://www.hei.org/htm/aemi.htm
Calvert, Dave 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 } -----------------------------------------------------------------------. } } } Listers } My company's safety folks are bent on making us wear Kevlar gloves while } razor trimming samples for ultramicrotomy - I'm talking about the final } trimming done using a trimming stand on the microtome. As you might know, } this is fine work - wearing gloves is a handicap. } My questions: } 1. Does anyone out there actually wear gloves? - if so then can you } recommend a glove? } 2. Are there other ways to make this task look less dangerous to the } safety police? (short of purchasing a trimming machine) } } Thanks! } } Dave Calvert } Eastman Chemical Company } Building 150B Lincoln Street (packages) } P.O. Box 1972 (US Mail) } Kingsport, Tennessee 37662-1972 } (423) 229-4943 } (423) 229-4558 fax } } } } } } RFC822 header } ----------------------------------- } } Received: from ultra5.microscopy.com [206.69.208.10] by mailhouse.hei.org } with ESMTP } (SMTPD32-6.00) id A8F3168B0262; Wed, 10 Jan 2001 22:55:47 -0800 } Received: (from daemon-at-localhost) } by ultra5.microscopy.com (8.9.3+Sun/8.9.1) id SAA00552 } for dist-Microscopy; Wed, 10 Jan 2001 18:06:37 -0600 (CST) } Received: from no_more_spam.com (sparc5 [206.69.208.10]) } by ultra5.microscopy.com (8.9.3+Sun/8.9.1) with SMTP id SAA00549 } for "MicroscopyFilteredEmail1-at-msa.microscopy.com"; Wed, 10 Jan 2001 } 18:06:07 -0600 (CST) } Received: from [206.69.208.21] (mac21.zaluzec.com [206.69.208.21]) } by ultra5.microscopy.com (8.9.3+Sun/8.9.1) with ESMTP id SAA00542 } for {Microscopy-at-MSA.Microscopy.Com} ; Wed, 10 Jan 2001 18:05:55 -0600 (CST) } X-Sender: zaluzec-at-ultra5.microscopy.com } Message-Id: {v03130301b682a8bd6c36-at-[206.69.208.21]} } Mime-Version: 1.0 } Content-Type: text/plain; charset="us-ascii" } Date: Wed, 10 Jan 2001 18:03:27 -0600 } To: Microscopy-at-sparc5.microscopy.com } From: "Calvert, Dave" {calvert-at-eastman.com} } Subject: Ultramicrotomy safety issues } Errors-to: Microscopy-request-at-sparc5.microscopy.com } X-RCPT-TO: {pwebster-at-hei.org} } X-UIDL: 273278871 } Status: R }
by ultra5.microscopy.com (8.9.3+Sun/8.9.1) id LAA02680 for dist-Microscopy; Thu, 11 Jan 2001 11:45:47 -0600 (CST) Received: from no_more_spam.com (sparc5 [206.69.208.10]) by ultra5.microscopy.com (8.9.3+Sun/8.9.1) with SMTP id LAA02677 for "MicroscopyFilteredEmail1-at-msa.microscopy.com"; Thu, 11 Jan 2001 11:45:17 -0600 (CST) Received: from utilitysrvr.qdots.com ([207.33.253.219]) by ultra5.microscopy.com (8.9.3+Sun/8.9.1) with ESMTP id LAA02670 for {Microscopy-at-MSA.Microscopy.Com} ; Thu, 11 Jan 2001 11:45:06 -0600 (CST) Received: by UTILITYSRVR with Internet Mail Service (5.5.2448.0) id {CN74FMKY} ; Thu, 11 Jan 2001 09:25:52 -0800 Message-ID: {4B747C1B1138D211B9DB0008C7BF0B242E026F-at-UTILITYSRVR}
Dear Colleagues,
Does anyone know any place that has a TEM with a dedicated STEM unit attached. The reason for the question is that I have particles composed of cores and shells (coated particles), both of which are different materials. By TEM I am not able to discern the shells from the cores because the contrast is extremely low. However, I am told that a dedicated STEM unit might allow me distinguish the shells from the cores based on the fact that they both have very different z-contrast.
Regards, Thearith
_________________________
Thearith Ung, Ph.D. Quantum Dot Corporation 26136 Research Road Hayward CA 94545 Tel: (510)-887-8775 (x4125) Fax:(510)-783-9729 www.qdots.com
Hi, I'm looking for technical assistance or a service manual for a Leitz Orthomat E (7916) Photo System.The problem we are having is the unit will not allow a picture to be taken unless there is very little light. Once the system thinks it is in range, there is not enough light present to get the photograph. An adjustment of the light detector? Any assistance is appreciated. Lewis McCrigler Humboldt State University
I've never worked with ink samples, but nevertheless I am trying to give some advice (be cautious!).
I think that techniques like freeze fracturing are not suitable for your purposes. Cracks could prefer to propagate through pores, so fracture surface will exaggerate porosity. Polished cross sections are much better for quantification. Maybe you could find suitable media for embedding. And what about mounting 2-3 substrates in a clip and cutting them with a sharp blade (hm... I really do not know ink's properties...)?
Vladimir
Vladimir M. Dusevich, Ph.D. Electron Microscope Lab Manager 3127 School of Dentistry 650 E. 25th Street Kansas City, MO 64108-2784
} -----Original Message----- } From: Tiffany Argent [mailto:tiffany.argent-at-abbott.com] } Sent: Thursday, January 11, 2001 6:07 AM } To: Microscopy-at-sparc5.microscopy.com } Subject: Cross section sample preparation } } } -------------------------------------------------------------- } ---------- } 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 trying to find a way of looking at a cross section of a } printed ink } approx 10um thick on a PVC substrate. I am trying to measure } the porosity of } the ink so I guess some image analysis will be used. It is } mainly a method } of preparing the samples that has me a bit stumped. I have } tried freeze } fracturing and embedding the samples in resin then polising } the surface. } Neither are satisfactory. The microscopy techniques I have } available are } SEM and LM. Can anyone help? }
One of our investigators is studying the ratio of total and phosphorylated transcription factor in the cell. We are able to do multiple fluorescence labeling but I need help in determining the fluorescence intensity ratios. We are using the Alexa dyes 350, 488 and 630 just to make sure there is no bleed through with the filters that we use. I would like to know if anyone has done this type of experiment and what are the potential problems that one could run into. I would appreciate comments or suggestions.
Thank you,
Cora Bucana Corazon D. Bucana, Ph.D. Dept. Cancer Biology UT M.D.Anderson Cancer Center 1515 Holcombe Blvd, Box 173 Houston, Texas 77030 Phone: 713-792-8106 FAX 713-792-8747
We've only lost about 4 technologists due to them accidentally cutting open their jugulars with a razor blade whilst trimming blocks and bleeding to death on the spot. So with that good safety record, we've chosen to dispense with the gloves thus far. Should we lose a few more though, the issue might come up again.
Garry
Charge Technologist - Electron Microscopy Department of Pathology Health Sciences Centre Winnipeg, Canada
I've never done any serious particle arranging, but perhaps one of the people mentioned below can help you.
You might try asking Klaus Kemp via the website at http://www.diatoms.co.uk since he creates arranged slides as a profession. He has been referred to as a master of the art at several microscopy seminars I've attended.
http://www.microscopy-uk.org.uk/mag/artapr00/machslide.html will take you to an article titled "A microscopical view of an old diatom circle pattern slide with 250+ diatom shells" by Martin Mach (there is a link to his e-mail). He provides a "Modern Microscopy" reference for preparation of such slides, but unless you have a GOOD library, you might ask him if he could send you a copy of the article - it is dated 1895.
Anna Teetsov at McCrone Associates (http://www.mccrone.com/ma/staff.html) is also expert at positioning particles on slides. While she is famous for manipulating the tiniest of particles, I've seen some beautiful arranged butterfly scale slides she's made for viewing under the light microscope. She might be willing to provide some suggestions.
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
jmkrupp-at-cats. ucsc.edu (Jon To: Microscopy-at-sparc5.microscopy.com Krupp) cc: Subject: Mounting large diatoms? 2001/01/10 03:54 PM
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Hi:
Does anyone know how to mount large (100um+) diatoms for LM or SEM? The little ones are OK, they stick to most any stub, but these big guys like to fall off.
Anyone know how arranged diatom slides are/were made? I checked WWW but no specifics on techniques. Something like these methods would work for us.
Thanks
Jonathan Krupp Microscopy & Imaging Lab University of California Santa Cruz, CA 95064 (831) 459-2477 jmkrupp-at-cats.ucsc.edu
A colleague (visiting from Brazil) is looking for a microtome for cutting semi-thin (0.25 to 2 micrometer) sections of plastic (epoxy) embedded specimens (mammalian tissues). He is considering a new Leica RM2165 ($18K).
I am soliciting testimonials (good and bad) for this or ANY other microtomes for cutting semi-thins.
Thank you on his behalf.
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/departments/shops/cem.html ##############################################################
We've solved that problem with Kevlar collars. We found that gloves just made it MORE likely that jugulars would be severed, so we don't use them either.
Randy
-----Original Message----- } From: Garry Burgess [mailto:GBurgess-at-exchange.hsc.mb.ca] Sent: Thursday, January 11, 2001 1:19 PM To: microscopy-at-sparc5.microscopy.com
We've only lost about 4 technologists due to them accidentally cutting open their jugulars with a razor blade whilst trimming blocks and bleeding to death on the spot. So with that good safety record, we've chosen to dispense with the gloves thus far. Should we lose a few more though, the issue might come up again.
Garry
Charge Technologist - Electron Microscopy Department of Pathology Health Sciences Centre Winnipeg, Canada
In my 21 years of thin sectioning I have from time to time cut my fingers, but a band aid is all that was needed. Kevlar gloves sound to me like ridiculous over kill. However for those of us working in really big and not always friendly cities, there might be an argument for Kevlar vests. Happy sectioning, Tim
Timothy G. Schneider Director of Electron Microscopy Department of Pathology Room 229 Jefferson Hall Thomas Jefferson University 1020 Locust St. Philadelphia Pa. 19107 215-503-4798 work 610-613-8170 cellular timothy.schneider-at-mail.tju.edu
----- Original Message ----- } From: "Garrison, Becky" {becky.garrison-at-jax.ufl.edu} } I have always worn latex gloves more for protection ( abrasion from } tightening chucks, etc.) Using long single edge razors (Weck Extra Long } Blades, EMS #71933-60) seems to give me more control of the blade and } therefore less of a chance to knick one's fingers. } I have at times shaved with a straight razor and that is little different that what a long single edge razor. Some people that have beards still do although a old Gillette safety razor with the guard removed is easier to use since sharpening a straight razor is a pain. Explaining that some folks still use them to shave should at least catch the safely Nazi off guard if not convince him of the absurdity of his request.
Gordon Gordon Couger gcouger-at-couger.com Stillwater, OK www.couger.com/gcouger 405 624-2855 GMT -6:00
Hi! I am interested in using a light microscope to digitize photographic film, i.e. to use my light microscope as a film scanner to scan negatives.
Since our lab does a fair amount of investigation into telepathology applications, we have scopes that are set up for the automatic scanning of multiple fields, merging of fields, etc. That problem is (relatively) solved.
What I am getting stumped on here is how to mount my 35mm photographic negatives. If I just slap one on a slide and set a coverslip on top, I get (not surprisingly) nontrivial refractive problems with irregularities in the surface of the film.
Unfortunately, these are photographic negatives which might have forensic/evidentiary value, so I can't dribble on any of the mounting media I can think of -- since I can't permanently mount the negative. I have to be able to take that negative at a later time and make an "original" photograph.
Anybody have experience with this? Any lore would be appreciated.
A one day TEM course sponsored by the AVS will given during the upcoming February Santa Clara meeting. For more information please see www.vacuum.org
At 9:04 AM -0800 12/13/00, Thearith H. Ung wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Glycerin has about the right refractive index and is easily washed out with water, after which the negatives can be air dried. Certainly glycerin works as a temporary mountant for microscope slides and the negative's gelatin emulsion is not affected by it. Cheers Jim Darley ProSciTech Microscopy PLUS PO Box 111, Thuringowa QLD 4817 Australia Ph +61 7 4774 0370 Fax:+61 7 4789 2313 service-at-proscitech.com Great microscopy catalogue, 500 Links, MSDS, User Notes ABN: 99 724 136 560 www.proscitech.com
On Friday, January 12, 2001 5:30 AM, William R. Oliver [SMTP:oliver-at-cpt.afip.org] wrote: } } } } Hi! I am interested in using a light } microscope to digitize photographic film, i.e. } to use my light microscope as a film scanner } to scan negatives. } } Since our lab does a fair amount of investigation } into telepathology applications, we have scopes } that are set up for the automatic scanning of } multiple fields, merging of fields, etc. That } problem is (relatively) solved. } } What I am getting stumped on here is how to } mount my 35mm photographic negatives. If I } just slap one on a slide and set a coverslip } on top, I get (not surprisingly) nontrivial } refractive problems with irregularities in the } surface of the film. } } Unfortunately, these are photographic negatives } which might have forensic/evidentiary value, so } I can't dribble on any of the mounting media I } can think of -- since I can't permanently mount } the negative. I have to be able to take that } negative at a later time and make an "original" } photograph. } } Anybody have experience with this? Any lore } would be appreciated. } } } billo } }
Don't do it. The reason for pumping detectors first without heat is to avoid further contamination of the crystal. When the dewar is heated material is released from the walls of the contained space and especially the molecular sieve. Pump first and then heat, that way the pump can cope and quickly eliminate the additional contaminants. Cheers Jim Darley ProSciTech Microscopy PLUS PO Box 111, Thuringowa QLD 4817 Australia Ph +61 7 4774 0370 Fax:+61 7 4789 2313 service-at-proscitech.com Great microscopy catalogue, 500 Links, MSDS, User Notes ABN: 99 724 136 560 www.proscitech.com
On Friday, January 12, 2001 2:28 AM, Faerber Jacques [SMTP:Jacques.Faerber-at-ipcms.u-strasbg.fr] wrote: } } Hello } } I have no experience in EDS detector pumping, but a little bit in vacuum } technology. } } What do you think about heating the Dewar before pumping ? } } That's what I do with sorbtion (zeolite) pumps used to prepump UHV vessel } (to have a dry pumping before starting turbo or ion pump). I put a heater } around the pump -in our case it would be hot water (hot air ? hot oil ? } which temperture can support the Dewar assembly ?)- let it warm over the } night, and close the venting valve. } } You could do something similar with the detector : warm it at air } pressure for a few hours (it schould dry too the zeolite) and than pump } down with turbo, but pre-pump with dry backing pump to prevent oil } contamination, } as Jim mentioned. Than pump down until the Dewar is cold, with a base } pressure of something like 10E-5 Torr. And after that, cool it with } nitrogen. } } What do you think about that ? } } Bye } } } J. Faerber } IPCMS-GSI } (Institut de Physique et Chimie des Materiaux de Strasbourg } Groupe Surface et Interfaces) } 23, rue de Loess } 67037 Strasbourg CEDEX } France } } Tel 00 33(0)3 88 10 71 01 } Fax 00 33(0)0 88 10 72 48 } E-mail Jacques.Faerber-at-ipcms.u-strasbg.fr
There is also a film cleaning fluid I found several at Porters Camera http://www.porters.com/ and search for "film cleaner" in their on line store. These usually don't require washing and would be easier to clean off than Glycerin. There is a scratch remover that might also work. I couldn't find it so it may have had something in it that the EPA didn't like. Your darkroom or local camera store may have these.
Gordon Gordon Couger gcouger-at-couger.com Stillwater, OK www.couger.com/gcouger 405 624-2855 GMT -6:00 } From: "Jim at ProSciTech" {jim-at-proscitech.com} } } Glycerin has about the right refractive index and is easily washed out with } water, after which the negatives can be air dried. Certainly glycerin works as } a temporary mountant for microscope slides and the negative's gelatin emulsion } is not affected by it. } Cheers } Jim Darley } ProSciTech Microscopy PLUS } PO Box 111, Thuringowa QLD 4817 Australia } Ph +61 7 4774 0370 Fax:+61 7 4789 2313 service-at-proscitech.com } Great microscopy catalogue, 500 Links, MSDS, User Notes } ABN: 99 724 136 560 www.proscitech.com } } On Friday, January 12, 2001 5:30 AM, William R. Oliver } [SMTP:oliver-at-cpt.afip.org] wrote: } } } } } } } } Hi! I am interested in using a light } } microscope to digitize photographic film, i.e. } } to use my light microscope as a film scanner } } to scan negatives. } } } } Since our lab does a fair amount of investigation } } into telepathology applications, we have scopes } } that are set up for the automatic scanning of } } multiple fields, merging of fields, etc. That } } problem is (relatively) solved. } } } } What I am getting stumped on here is how to } } mount my 35mm photographic negatives. If I } } just slap one on a slide and set a coverslip } } on top, I get (not surprisingly) nontrivial } } refractive problems with irregularities in the } } surface of the film. } } } } Unfortunately, these are photographic negatives } } which might have forensic/evidentiary value, so } } I can't dribble on any of the mounting media I } } can think of -- since I can't permanently mount } } the negative. I have to be able to take that } } negative at a later time and make an "original" } } photograph. } } } } Anybody have experience with this? Any lore } } would be appreciated. } } } } } } billo } } } } } }
does anybody knows the telephone number from Biosupplies (Melbourne, Australia), I bought a callose ((1-3)beta-glucan-specific) monoclonal antibody two years ago and I can't contact with them at the telephone that I have. Thanks a lot Nuria
------------------------------------------------------------------------------ Nuria Cortadellas Unitat de Microscopia de Transmissio Serveis Cientifico-Tecnics Universitat de Barcelona C/ Sole i Sabaris, 1-3 08028 Barcelona Tel: +34 3 402 13 52 Fax: +34 3 402 13 98 E-mail: nuriac-at-giga.sct.ub.es
We put up with the minor wounds. I do however tell students not to cut themselves as I will be obliged to fill in an accident form and the safety officer will invite me to think of alterative methods. We thought of blunting the blade corners or making little corner guards but never got round to it.
Dave
On Thu, 11 Jan 2001 15:50:36 -0500 Timothy Schneider {Timothy.Schneider-at-Mail.TJU.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 } -----------------------------------------------------------------------. } } } Dave: } } In my 21 years of thin sectioning I have from time to time cut my fingers, } but a band aid is all that was needed. Kevlar gloves sound to me like } ridiculous over kill. However for those of us working in really big and not } always friendly cities, there might be an argument for Kevlar vests. Happy } sectioning, Tim } } Timothy G. Schneider } Director of Electron Microscopy } Department of Pathology } Room 229 Jefferson Hall } Thomas Jefferson University } 1020 Locust St. } Philadelphia Pa. 19107 } 215-503-4798 work } 610-613-8170 cellular } timothy.schneider-at-mail.tju.edu } }
---------------------------------------- Patton, David Email: David.Patton-at-uwe.ac.uk "University of the West of England"
we use a Hitachi H7000 with STEM attachment although I'm sure there will be someone much closer to you, but I would like to make a couple of comments: you mention a dedicated STEM unit which to me is a free-standing high resolution STEM and not a STEM attachment to a TEM. There should be lots of TEMs with STEM attachments on instruments bought in the last 10 or 15 years but only a few high resolution STEMs because they are expensive and specialized (try Brookhaven National Laboratory website http://bnlstb.bio.bnl.gov/biodocs/stem/stem.htmlx).
You may also want to consider that certain TEMs have built in energy filtering or electron energy spectrometers which can actually be tuned for different atomic masses in the specimen - Zeiss EM902s can do this but I'm not sure if any other machines are available.
I have no connection with Brookhaven or Zeiss, although of course I do use Hitachi.
Good luck
Malcolm
Malcolm Haswell e.m. unit University of Sunderland UK
"Thearith H. Ung" 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 Colleagues, } } Does anyone know any place that has a TEM with a dedicated STEM unit } attached. The reason for the question is that I have particles composed of } cores and shells (coated particles), both of which are different materials. } By TEM I am not able to discern the shells from the cores because the } contrast is extremely low. However, I am told that a dedicated STEM unit } might allow me distinguish the shells from the cores based on the fact that } they both have very different z-contrast. } } Regards, } Thearith } } _________________________ } } Thearith Ung, Ph.D. } Quantum Dot Corporation } 26136 Research Road } Hayward CA 94545 } Tel: (510)-887-8775 (x4125) } Fax:(510)-783-9729 } www.qdots.com
Glycerin, and also ethylene glycol, can be dried under vacuum making it possible to avoid rehydrating the negative Chris
----- Original Message ----- } From: "Jim at ProSciTech" {jim-at-proscitech.com} To: "'William R. Oliver'" {oliver-at-cpt.afip.org} ; {microscopy-at-sparc5.microscopy.com} Sent: Friday, January 12, 2001 12:52 AM
Before this subject is banned from the list -
Our only serious injuries to date are blinded students falling asleep while sectioning and poking their eyes out on the binocular eyepieces!
Perhaps the kevlar collars would keep their heads up a little longer?!
Pete
-- Peter Bond Plymouth Electron Microscopy Unit University of Plymouth Drake Circus Plymouth Devon UK PL4 8AA Tel/Fax: 01752 233092 email: pbond-at-plymouth.ac.uk
I am trying to judge the optical quality of two similar stereoscopic zoom scopes: the Nikon SMZ800 and the Leica MZ7, both equipped with a 1x Planapochromatic objective.
Leica publishes resolution figures for the MZ7, claiming 309 line pairs per mm. Nikon does not, and I haven't been able to persuade the Nikon representative to "characterize" the resolution of the SMZ800, although he says he can. I do not have the necessary test slide, nor do I know where I can get one with a scale graduated from say 200-400 lp/mm. I do know though that such a slide would cost probably $300-$500.
Interestingly, Nikon publishes a resolution number for its next higher quality scope, the SMZ1000. It claims the SMZ1000 can resolve 300 lp/mm with a 1x Planapo. Because Nikon product literature doesn't publish a resolution for the SMZ800, I suspect that its resolution is substantially lower than 300 lp/mm, and therefore inferior to the Leica MZ7.
Does anyone have any suggestions on how I might judge the relative quality of these two scopes, or does anyone have experience with either scope that might shed light on this problem? Is my only alternative to find and buy a suitable test slide? If so, can anyone point me to a source?
Thanks very much, Ed
Ed Bachmann Odum Institute for Research in Social Science Manning Hall CB 3355 University of North Carolina at Chapel Hill Chapel Hill, NC 27599-3355 (919) 962-0512
Here are a couple of references you might find useful, from a specialist on this kind of electron microscopy. I'll send the abstracts as attachments separately.
Srnova-Sloufova I, Lednicky F, Gemperle A, et al. Core-shell (Ag)Au bimetallic nanoparticles: Analysis of transmission electron microscopy images LANGMUIR 16: (25) 9928-9935 DEC 12 2000
Lednicky F, Coufalova E, Hromadkova J, et al. Low-voltage TEM imaging of polymer blends POLYMER
} "Thearith H. Ung" wrote: } } } } Dear Colleagues, } } } } Does anyone know any place that has a TEM with a dedicated STEM unit } } attached. The reason for the question is that I have particles composed of } } cores and shells (coated particles), both of which are different materials. } } By TEM I am not able to discern the shells from the cores because the } } contrast is extremely low. However, I am told that a dedicated STEM unit } } might allow me distinguish the shells from the cores based on the fact that } } they both have very different z-contrast. } } } } Regards, } } Thearith } } } } _________________________ } } } } Thearith Ung, Ph.D. } } Quantum Dot Corporation } } 26136 Research Road } } Hayward CA 94545 } } Tel: (510)-887-8775 (x4125) } } Fax:(510)-783-9729 } } www.qdots.com
+------------------------------------------------------------------------+ | Robert H.Olley Phone: | | J.J.Thomson Physical Laboratory {direct line +44 (0) 118 9318572 | | University of Reading {University internal extension 7867 | | Whiteknights Fax +44 (0) 118 9750203 | | Reading RG6 6AF Email: R.H.Olley-at-reading.ac.uk | | England URL: http://www.reading.ac.uk/~spsolley | +------------------------------------------------------------------------+
Abstract: Layered core-shell bimetallic silver-gold colloids in the size range of 10-16 nm have been prepared by the seed-growth method. Silver nuclei were covered by gold shells of various thicknesses without any stabilization agent. Interfacial (Ag)Au colloid-2,2'-bipyridine films were prepared from these bimetallic colloids and used for the purpose of analysis of transmission electron microscopy (TEM) images and electron diffraction. Both observed and calculated TEM images were used to characterize the prepared nanoparticles. On the basis of the analysis of TEM images, the calculated TEM image contrast, and results obtained by electron diffraction, energy-dispersive X-ray analysis, and other experiments, the core-shell structure of the prepared (Ag)Au nanoparticles was revealed. Particles were found to consist of a silver core and a gold shell enriched with silver.
Abstract: Low-voltage transmission electron microscopy (LV-TEM) was applied to obtain images of the phase structure of selected polymer blends without any prior staining. The instrument used (LVTEM-5, working at 5 kV) is of a novel construction combining visual-light and electronmicroscopical techniques, resulting in an enhanced efficiency of light transport to the eye and facilitating CCD imaging. Results were compared wi th LV-STEM at 25 kV. Phase structure of polycarbonate/poly( styrene-co-acrylonitrile) (PC/SAN), polystyrene/polypropylene (PS/PP), and polyethylene/polypropylene blends (PE/PP, ADFLEX) were selected to demonstrate the above techniques. The difference in density between the individual components of polymer blends was found to be the reason for the obtained image contrast. Differences less than 0.04 g/cm(3) can be traced with this technique.
First off, I can't understand the rationale for using an LM to do neg scanning. Why not just use a scanner? Easy, fast, reproducable.
If you do want to use an LM, it seems to me that a low power objective is required in order to avoid imaging mostly the grain structure. With a typical field of view for the camera, you will likely be taking about 100 individual shots and then stitching them together. A 2.5X objective works on low NA condensers. A 1X objective requires an ultra low condenser. But even this would result in a 10X FOV on each image frame.
Notwithstanding the above, if you do want to temporarily mount 35mm frames, get Bair mounts from the Stock Solution, Salt Lake City.
http://www.tssphoto.com/sp/index.html
These are self-adhesive cardboard mounts which stick to themselves but not to the film. When you are done, just peel the mount apart and your neg will fall out.
gary g.
http://photoweb.net
At 11:29 AM 1/11/01, you wrote:
} Hi! I am interested in using a light } microscope to digitize photographic film, i.e. } to use my light microscope as a film scanner } to scan negatives. } } Since our lab does a fair amount of investigation } into telepathology applications, we have scopes } that are set up for the automatic scanning of } multiple fields, merging of fields, etc. That } problem is (relatively) solved. } } What I am getting stumped on here is how to } mount my 35mm photographic negatives. If I } just slap one on a slide and set a coverslip } on top, I get (not surprisingly) nontrivial } refractive problems with irregularities in the } surface of the film. } } Unfortunately, these are photographic negatives } which might have forensic/evidentiary value, so } I can't dribble on any of the mounting media I } can think of -- since I can't permanently mount } the negative. I have to be able to take that } negative at a later time and make an "original" } photograph. } } Anybody have experience with this? Any lore } would be appreciated. } } } billo
Some things don't need solvents. For example, citric acid can be melted on a hotplate at about 100^C, and if cooled slowly will give chunky crystals in all sorts of birefringence colours.
If you have a hot enough plate, it's good to look at sodium nitrate (mp about 305^C. This will form large slabs of crystals. These don't look so good in themselves, but if you have a Bertrand lens or else simply pull out the eyepiece and look at down the tube, many of them will display concentric rings on a Maltese cross, the interference pattern resulting from different path lengths of the two polarized rays through the crystal. Try this with different magnification objectives. The citric acid will also give wonderful interference patterns, but they're much more complicated.
Other organic compounds can simply be melted, and when cooled between cover slip and hot plate will form spherulites.
If you melt a thin film of polypropylene between slide and cover slip, and cool slowly, you will get fantastic spherulites. Spherulites are found in many plastics, but polypropylene is the star performer. (Further details on request).
+------------------------------------------------------------------------+ | Robert H.Olley Phone: | | J.J.Thomson Physical Laboratory {direct line +44 (0) 118 9318572 | | University of Reading {University internal extension 7867 | | Whiteknights Fax +44 (0) 118 9750203 | | Reading RG6 6AF Email: R.H.Olley-at-reading.ac.uk | | England URL: http://www.reading.ac.uk/~spsolley | +------------------------------------------------------------------------+
On Fri, 5 Jan 2001 us004118-at-mindspring.com wrote:
} Question: I am enjoying doing photomicrographs of crystal preparations } in polarized light. However I have insuffient knowledge of chemistry to } choose solvents without a long series of trial and error efforts.Can you } give me a rationale and/or a reference to go about this in a more } productive manner?
Email: us004118-at-mindspring.com Name: Leonard Lessin, FBPA
*************************************************** Last call for papers: FOCUS ON MICROSCOPY 2001 ***************************************************
FOM 2001 , Amsterdam The Netherlands, April 1-4, 2001
FOM 2001 is a world leading international conference on advanced microscopy. It is the joint meeting of the 13th International Conference on Confocal Microscopy and the 13th International Conference on 3D Image Processing in Microscopy.
FOM 2001 will be held at the Academic Medical Centre (AMC) of the University of Amsterdam, Amsterdam, The Netherlands.
For more information visit: http://www.focusonmicroscopy.org
Call for abstracts ------------------ Deadline for abstract submission: february 1st, 2001.
Core conference subjects: "INSTRUMENTATION" and "IMAGE PROCESSING AND ANALYSIS"
SPEAKERS: S. Hell (Gottingen, Germany), T. Wilson (Oxford, UK), S. Kawata (Osaka, Japan) C.J.R. Sheppard (Sydney, Astralia), C. Coggswell (Sydney, Astralia) E. Stelzer (Heidelberg, Germany) C. Cremer (Heidelberg, Germany), P.A. Benedetti (Pisa, Italy), A. Kriete (Giessen, Germany), H. van der Voort (Hilversum, The Netherlands), P.C. Cheng (Buffalo, USA), G.J. Brakenhoff (Amsterdam, The Netherlands)
Special conference subjects this year: MULTI-PHOTON MICROSCOPY" and "MICROSCOPY OF LIVING CELLS AND TISSUE".
SPEAKERS: A. Zumbusch (Muenchen, Germany), L. Moreaux (Paris, France) A. Diaspro (Genova, Italy), M. Muller (Amsterdam, The Netherlands), K. Sullivan (La Jolla, USA, to be confirmed), R. van Driel (Amsterdam, The Netherlands), R. Eils (Heidelberg, Germany), T. Mistelli (Bethesda, USA; to be confirmed), D. Gadella (Wageningen, The Netherlands), J. Dobrucki (Krakov, Poland), A. Houtsmuller (Rotterdam, The Netherlands), E. Manders (Amsterdam, The Netherlands)
} First off, I can't understand the rationale for using an } LM to do neg scanning. Why not just use a scanner? } Easy, fast, reproducable.
There are a couple. The driving reason for me is that this gives me a *lot* more control in exploiting the lighting of the negative.
I do forensic image processing as well as "regular" pathology stuff. Consider the following scenario:
A bad guy is sitting in a shadowed room aiming a rifle through a window. Joe Snuffy tourist takes a photo of the street which incidentally captures the window (let's assume that Joe Snuffy is a purist and isn't using a Mavica, in which this is all moot and useless). The window is largely a dark blob.
The task, then is to get as much information of that dark blobby window as possible. If you look at most film scanners on the market, particularly in any reasonable price range, you don't have the option of cranking your illumination up or down, of sticking filters in the light pathway, of doing all the stuff we take for granted as microscopists.
There's a lot of tools in them thar microscopy hills. It ain't so, it seems, with the film scanners I have available.
Instead, almost always, the only thing you can play with is the gamma. That means you are going to spend a lot of your representation space on stuff you don't want to see. The scanner is going to get two bits of data out of that blob, whatever knob you twiddle.
Playing games resetting the gamma as an option in a TWAIN driver won't fix this, and I haven't seen a "burn the bejezus out of this little area here and ignore the rest of the slide" button. Oh, sure, you can take those two bits the scanner gives you and display it as 0 and 1 or 0 and 255, but it ain't going to fill up the space in between. Not even with noise. The bottom line is that my impression is that film has dynamic range that is not accessible to most film scanners.
As a secondary issue, I have a few ideas for for playing with grain and restoration that might benefit from data aquisition at a higher resolution.
} } If you do want to use an LM, it seems to me that a low } power objective is required in order to avoid imaging } mostly the grain structure.
Sorta, but I am actually interested in seeing about characterizing the grain structure and seeing if that characterization can be useful in restoration.
Finally, I have a good characterization of the mtf of my microscope. I don't have a good characterization of the mtf of my flatbed scanner. While that doesn't help me with blind deconvolution for the camera mtf, it does help me for at least that part of the restoration of the image. I may be goofy, but I'd like to play with it a little.
If you have some experience with this, I'd love to learn from you. I figure that *somebody* must have played with this, but I haven't been able to find much literature on it. Do you have some lore you would like to share (nudge, nudge)?
} With a typical field of view } for the camera, you will likely be taking about 100 } individual shots and then stitching them together.
Something like that. But that stitching and data handling is something we do on a daily basis.
} } Notwithstanding the above, if you do want to temporarily } mount 35mm frames, get Bair mounts from the Stock } Solution, Salt Lake City. } } http://www.tssphoto.com/sp/index.html
} Does anyone know any place that has a TEM with a dedicated STEM unit } attached. The reason for the question is that I have particles composed } of cores and shells (coated particles), both of which are different } materials. } By TEM I am not able to discern the shells from the cores because the } contrast is extremely low. However, I am told that a dedicated STEM unit } might allow me distinguish the shells from the cores based on the fact } that they both have very different z-contrast.
I agree with the person who suggested an energy-filtering TEM, such as the Zeiss 902. We have the newer version, the LEO 912, and I have also been doing some work with coated nanoparticles. Yes, it is possible to see the difference between the cores and coating with this type of instrument.
Aloha, Tina
http://www.pbrc.hawaii.edu/bemf/microangela
**************************************************************************** * Tina (Weatherby) Carvalho * tina-at-pbrc.hawaii.edu * * Biological Electron Microscope Facility * (808) 956-6251 * * University of Hawaii at Manoa * http://www.pbrc.hawaii.edu/bemf* ****************************************************************************
Someone here would like to probe for heparin on some amyloid fibrils they have made. Fibril formation is different in the presence of heparin and they are curious to know if the heparin is binding to the fibrils or not.
They prepare the fibrils in their lab, don't ask me how, and apply liquid suspensions to a formvar coated grid. We negative stain with UA and then go to the TEM to look for fibrils.
The results of the neg stain search can be variable, sometimes the fibrils look like fibers, other times it seems to be just a bunch of junk, so the fibril formation is not always we defined. These folks are trying to figure out whether to probe the fibrils on the grid, or before while still suspended. But they tell me that often the fibrils do not survive too many washings in suspension, so maybe probing in solution before applying to grids could be a problem.
Any ideas, this is not my area of expertise.
Thanks
Jonathan Krupp Microscopy & Imaging Lab University of California Santa Cruz, CA 95064 (831) 459-2477 jmkrupp-at-cats.ucsc.edu
Food Structure & Functionality Symposium 2001 An international symposium leading food structure & Functionality studies through the 21st century *webaddress at the AOCS site http://www.aocs.org/member/division/fsff/index.htm*
Being held in conjunction with the , May 13-16, 2001, Minneapolis Convention Center, Minneapolis, Minnesota, USA. For information, e-mail us at: meetings-at-aocs.org
The symposium has two themes: * New and novel approaches (including microscopy, rheology and spectroscopy) to the study of structure-function relationships in foods; * Food system studies covering any part of the processing chain - from the raw material to the final product, and including trouble shooting.
Tentative Program (confirmed as of January 12th, 2001)
May 13th - Short Courses (short courses will run for a full day, and will run concurrently)
1) Food Contaminants. Contact person - Mark Auty 2) Specific Labeling in Foods. Contact person - Marcel Paques
May 14th-16th inclusive - Technical sessions 6 sessions will run over 3 days
Morning Symposium opening Plenary lecture - Food Quality andwhy the Structure matters. P. Lillford, Unilever Research, Colworth House UK
Session 1: Dairy Products and Fat Based Foods Session - chairs M. Auty and M. Paques
Milk protein polysaccharide interactions in aqueous solutions and oil-in-water emulsions. H. Singh*, Y. Hemar & P. Munro, Institute of Food, Nutrition and Human Health Massey University, Palmerston North, New Zealand
Structural functions of dairy ingredients in products formulated with taro flour. C. Onwulata, USDA/ARS,Eastern Regional Research Center,Wyndmoor, PA 19038
Confocal imaging of galactomannan mode of action in recrystallisation of ice in model ice cream D. Ferdinando, Unilever Research Colworth House, UK
Heating of Food Proteins in a Closed System at High Temperature N. Kitabatake, Kyoto University, Japan
Milk Protein - molecular components and functional properties. N. C. Ganguli, Indian Dairy Association
Afternoon Session 2: Food Safety - chairs J. W. Arnold and R. Droleskey Prevention of Foodborne Illness Through Sanitation and Processing Technology J.W. Arnold; USDA/ARS, Russell Research Center; Athens, GA 30604
PreHarvest Intervention Strategies to Control Foodborne Pathogens in Poultry J. A. Byrd; USDA/ARS/SPARC; College Station, TX 77845
Interactions of Competitive Exclusion Cultures with the Intestinal Mucosa of Newly Hatched Chicks R. Droleskey; USDA/ARS/SPARC; College Station, TX 77845
Adhesion of Salmonella on Alfalfa Sprouts A. Chartowski; USDA/ARS, Western Regional Research Center; Albany, CA 94710
Growth of Fusarium moniliforme Dependent upon Corn Tissue Type I. E. Yates; USDA/ARS, Russell Research Center; Athens, GA 30604
Dedicated poster viewing 4:00-6:00PM
Evening: Round Table Discussion - topic to be announced
Tuesday, May 15th, 2001 Morning Session 3: New Methods and Techniques for Food Structure and Functionality Analysis -chair K.Groves
Diffusing wave spectroscopy - a new and non-invasive method for the investigation of the structure, dynamics and interactions in complex food systems M. Alexander* and P. Schurtenberger
Food: How complex can it be? E. Esselink ,Unilever Research Vlaardingen, The Netherlands
Immunolocalization of Transgenic Protein in Wheat Endosperm M. L. Parker *, E. Stoger, R. Casey and P. Christou, Institute of Food Research, Norwich, England.
Structure/Function relationships through microrheology. M. Paques, Wageningen Centre for Food Sciences/Unilever Research Vlaardingen
Specific labeling techniques for foods J. Leunissen, Aurion: Immuno-Gold Reagents & Accessories, The Netherlands
Food Structure and Functionality Division Luncheon. Dr. Brian Brooker (Institute of Food Research, England * retired) will be presented with the Food Structure and Functionality Division award and will give a presentation entitled: Fat crystals - the importance of being small.
Afternoon Session 4: Agricultural Applications of Microscopy and Imaging Session- chairs D.F.Wood and P. Allan-Wojtas
The Utility of Sorting in Agriculture. H. J. Arnott, Department of Biology, University of Texas at Arlington, Texas
The Potential for Automatic X-ray Sorting of Insect Infested Grain R. Haff . USDA - ARS - WRRC, Albany, California.
Automated Sorting of Almonds with Embedded Shell by Laser Transmittance Imaging T. Pearson* R. Young, USDA - ARS - WRRC, Albany, California.
Use of a GFP-transformed strain of Fusarium graminearum to study ear rot development in corn S. S. Miller. , AAFC - ECORC, Ottawa, Ontario, Canada.
Popping modifies endosperm structure and improves digestibility in maize and sorghum. M.L. Parker, Institute of Food Research, Norwich, England.
Microstructural Changes in Rice During Cooking D. Wood* and P.C. Yu . USDA - ARS - WRRC, Albany, California.
Evening: Food Structure and Functionality Division Member meeting
Wednesday, May 16th, 2001 Morning Session 5: Ingredients and Food Processing - chairs D. Kittleson and J. Charbonneau
Water continuous fat crystal networks in ice cream induced by unsaturated monoglycerides N. M. Barfod , Danisco Cultor, Brabrand, Denmark
High pressure application fo food systems and its impact on functional ingredients B. Tauscher*, P. Butz,and A.F. Garcia, Federal Research Center for Nutrition, Karlsruhe, Germany
Specificity and application of lipolytic enzymes in bread making processes T.B. Frandsen, T. Spendler, G. Budolfsen, L. Christiansen and J. B. Neilsen, Novozymes A/S, Bagsvaerd, Denmark
Afternoon Session 6: Colloidal and Interfacial Sciences - chairs D. Pechak and M. Paques
Rheology and Structure of Particulate Protein Gels T. van Vliet, Wageningen Centre for Food Sciences,Wageningen, The Netherlands
Posters:
1. In situ study of the effect of heating on dough components using Attenuated Total Reflectance-Fourier Transform Infrared (ATR-FTIR)
O. Sevenou, S.E. Hill, I.A. Farhat and J.R. Mitchell. Division of Food Sciences, University of Nottingham, Loughborough, UK
2. Antioxidative activity of the crude extract of lignan glycosides from sesame meal
Y-S Shue and L.S. Hwang, Graduate Institute of Food Science and Technology, National Taiwan University, Taiwan, R.O.C.
3. Near Field Microscopy of phase separation in a mixed interfacial protein/surfactant film
A. P. Gunning, A.R. Mackie, A.R. Kirby and V.J. Morris, Institute of Food Research, Norwich Research Park, Norwich, UK
Contact information for the chairs is shown below, in alphabetical order:
Paula Allan-Wojtas 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-em.agr.ca
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 email: jarnold-at-ars.usda.gov
Mark Auty Dairy Products Research Centre TEAGASC Moorepark, Femoy, Co. Cork Ireland Tel: 011-353-25-42447 FAX: 011-353-25-42340 email: mauty-at-moorepark.teagasc.ie
James E. Charbonneau National Food Processors Association Food Chemistry and Packaging Department 1401 New York Ave, NW Washington, D.C. 20005 USA Tel: (202) 639-5972 FAX: (202) 639-5991 email: jcharbo-at-nfpa-food.org
Kathy Groves Leatherhead Food Research Association Randalls Road, Leatherhead Surrey KT22 7RY England Tel: 44 0132 822330 FAX: 44 0132 386228 email: kgroves-at-lfra.co.uk
Tony McKenna New Zealand Dairy Institute Private Bag 11 029 Palmerston North, New Zealand Tel: 011 64 6 350 4649 FAX: 011 64 6 356 1476 email: tony.mckenna-at-nzdri.org.nz
Marcel Paques Wageningen Centre for Food Sciences/Unilever Research Vlaardingen P.O. Box 20, 6710 BA Ede The Netherlands Tel: 011 31 318 659690 FAX: 011-31-318 650400 email: paques-at-nizo.nl
David Pechak Kraft Technology Centre 801 Waukegan Road Glenview, IL 60025 USA Tel: (847) 646-4808 FAX: (847) 646-3864 email: dpechak-at-kraft.com
Delilah Wood USDA - ARS - WWRC 800 Buchanan Street Albany, CA 94710 USA Tel: (510) 559-5653 FAX: (510) 559-5777 email: wood-at-pw.usda.gov
Greetings, Does anyone have experience with lanthanum and/or ruthenium HT staining specifically for isolated cells?? I prepared two samples of single atrial cells, using protocols from the 60's and 70's. The ultrastructure was great, in part because I believe that the lanthanum as well as the ruthenium enhanced the UA and LC staining. I was hoping for a much more dense cell margin that would help to delineate vesicles that might be open to the surface. I know that Ruthenium HT is supposed to bind to the glycocalyx and stain well....but the lanthanum protocols I could find were all intact tissue where the spaces between cells were filled with dense material. I am not sure that lanthanum works for single cells, but gave it a try. Ruth. HT was added to both the GA and OsO4, but lanthamun was used, per protocol, only in the OsO4. Etoh dehydration and Embed 812 resin. Any sage wisdom on how to improve staining on a single cell prep would be helpful. Linda Fox lfox1-at-lumc.edu
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Fellow Microscopists: As many of you know, the Facility Management session held at M&M2000 was very well received and there was a unanimous request for it to be continued. Therefore a similar session will be held at M&M 2001. I must finalize the topics within the next week or two. Since the purpose of this session is to discuss topics of interest to facility managers, I would like your input before the session is finalized.
The topics covered in the M&M 2000 session with transcripts published in Microscopy Today were: 1) Multi-user Facilities...managing users 2) Justification of Costs, cost recovery, electronic bookkeeping and billing 3) Equipment Maintenance: Vender service contracts vs. Independent providers vs. Insurance company/self-insure options.
The following are some suggestions that were gleaned from the evaluation forms and discussion during the session.
1) Training Users…courses, workshops, …what works for whom? 2) Scientific Ethics…What are our responsibilities as lab Managers? 3) Mission statements/lab organization/lab business plans/future planning issues 4) Staffing issues including training, part-time student help, Training course T.A’s 5) Daily issues…prioritizing use, prioritizing service projects, dealing with difficult users/customers 6) Legal issues involving data ownership, confidentiality of data, handling of potential evidence. 7) Justification for new equipment 8) Commercial use of university facilities 9) Microscopy as a research tool…integration of industry or campus facilities in coordination with other core facilities. 10) Issues unique to Multi-user and/or Service facilities and how such facilities can coexist.
The first 2 received the greatest number of requests. However there may be more relevant topics now. Please rank the 3 of highest priority to you or suggest additional topics of interest. I will sift through all replies at the end of next week and narrow them down to 3. Also please feel free to supply the names of individuals to lead specific discussion topics. The format will be the same as the last session. A presenter will give a 10-15 min. introduction of the topic followed by ~30 min. open discussion.
Thanks, Debby
Debby Sherman Phone: 765-494-6666 Life Science Microscopy Facility FAX: 765-494-5896 Purdue University E-mail: dsherman-at-purdue.edu S-099e Whistler Building West Lafayette, IN 47907
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Hi All, On the "serious" side of this, and to make the safety police happy, EMS sells a plastic guard that holds razor blades, exposing just a small expanse for trimming. I had bought some years ago, on the "that sound good" premise. Personally, I found them awkward to use, but they are cheap, and having them in the lab (even if not used) may be enough to satisfy your safety wizards.
Disclaimer: I have no financial interests in EMS.
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
Mounting of particles on the order of 50-100um onto double stick tape is easily done as previously noted by using a very fine artist's brush and distilled water. But this should be done moist, rather than wet. After dipping the brush into DW, twirling the length of the brush end on a lab tissue both removes excess water and creates a finer point at the tip. The moist, fine-tipped brush can then not only pick up the diatom, foram or other particle, but can also be used to orient it and position it on the tape with good control. This method also prevents glue from bleeding up the particle. Particles of this size range can also be set down on a thin layer of silver conducting paint that's still wet, if you can chase the drying horizon fast enough, or on a thin layer of still-wet collodion (the same adhesive used by belly dancers to secure the navel jewel, but that's another story).
*************************************************************** Dee Breger Mgr. SEM/EDX Facility Lamont-Doherty Earth Observatory 61 Route 9W Palisades, NY 10964 USA T: 914/365-8640 F: 914/365-8155
http://www.ldeo.columbia.edu/micro http://www.discovery.com/area/science/micro/micro1.html http://www.lsc.org/antarctica/front.html Journeys in Microspace (Columbia University Press, 1995)
Ed: Edmund Scientific sells test slides for microscopes. Perhaps you can find an adequate one there. Some test slides run up $300, though. Or, what about using diatoms to compare one scope with another?
Sam Purdy Technical Center/National Steel Corp Trenton MI } ---------- } From: ed_bachmann-at-unc.edu } Sent: Friday, January 2001, 11:01 AM } To: microscopy-at-sparc5.microscopy.com } Subject: Nikon SMZ800 vs Leica MZ7 Stereozooms } } ------------------------------------------------------------------------ } 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 trying to judge the optical quality of two similar stereoscopic zoom } scopes: the Nikon SMZ800 and the Leica MZ7, both equipped with a 1x } Planapochromatic objective. } } Leica publishes resolution figures for the MZ7, claiming 309 line pairs } per mm. } Nikon does not, and I haven't been able to persuade the Nikon } representative to } "characterize" the resolution of the SMZ800, although he says he can. I } do not } have the necessary test slide, nor do I know where I can get one with a } scale } graduated from say 200-400 lp/mm. I do know though that such a slide } would cost } probably $300-$500. } } Interestingly, Nikon publishes a resolution number for its next higher } quality } scope, the SMZ1000. It claims the SMZ1000 can resolve 300 lp/mm with a 1x } Planapo. Because Nikon product literature doesn't publish a resolution } for the } SMZ800, I suspect that its resolution is substantially lower than 300 } lp/mm, and } therefore inferior to the Leica MZ7. } } Does anyone have any suggestions on how I might judge the relative quality } of } these two scopes, or does anyone have experience with either scope that } might } shed light on this problem? Is my only alternative to find and buy a } suitable } test slide? If so, can anyone point me to a source? } } Thanks very much, } Ed } } Ed Bachmann } Odum Institute for Research in Social Science } Manning Hall CB 3355 } University of North Carolina at Chapel Hill } Chapel Hill, NC 27599-3355 } (919) 962-0512 } }
I believe that the time-honoured method of manipulating small particles with a fine brush can be improved on. A customer thought that certain specimen should not be wetted, because they were to be weighed. Presumably they could be left to dry, but that was inconvenient. I suggested one of those vacuum pick-up devices; these pick up specimens using a square tipped syringe needle. Obviously those needles are too large for foramifera but they can be tipped with thin plastic tubing. On the first try I pulled some 0.3mm internal tubing using a PE transfer pipette. With practice smaller tubes could be produced. I suggest that manipulating specimens with a vacuum pick-up is faster and more precise than using a brush. I have used a vacuum pick-up for placing (and turning over) TEM grids when making support films. Its a rather more elegant and faster method than using tweezers. Disclaimer: ProSciTech is a supplier of vacuum pick-ups. Cheers Jim Darley ProSciTech Microscopy PLUS PO Box 111, Thuringowa QLD 4817 Australia Ph +61 7 4774 0370 Fax:+61 7 4789 2313 service-at-proscitech.com Great microscopy catalogue, 500 Links, MSDS, User Notes ABN: 99 724 136 560 www.proscitech.com
On Saturday, January 13, 2001 9:18 AM, Dee Breger [SMTP:micro-at-ldeo.columbia.edu] wrote: } } } Mounting of particles on the order of 50-100um onto double stick tape is } easily done as previously noted by using a very fine artist's brush and } distilled water. But this should be done moist, rather than wet. After } dipping the brush into DW, twirling the length of the brush end on a lab } tissue both removes excess water and creates a finer point at the tip. The } moist, fine-tipped brush can then not only pick up the diatom, foram or } other particle, but can also be used to orient it and position it on the } tape with good control. This method also prevents glue from bleeding up the } particle. Particles of this size range can also be set down on a thin } layer of silver conducting paint that's still wet, if you can chase the } drying horizon fast enough, or on a thin layer of still-wet collodion (the } same adhesive used by belly dancers to secure the navel jewel, but that's } another story). } } } *************************************************************** } Dee Breger } Mgr. SEM/EDX Facility } Lamont-Doherty Earth Observatory } 61 Route 9W } Palisades, NY 10964 USA } T: 914/365-8640 } F: 914/365-8155 } } http://www.ldeo.columbia.edu/micro } http://www.discovery.com/area/science/micro/micro1.html } http://www.lsc.org/antarctica/front.html } Journeys in Microspace (Columbia University Press, 1995) } }
Hi Listers, I've been thrown on the scrapheap at 60. So I'll be unsubscribing soon but will keep an eye on the list over a colleague's shoulder. Many thanks for all the help and interesting items, especially the forensic stuff - a fascinating and useful insight into the problems of others. Byeeee, Chris, Plant Path., IACR-Rothamsted, UK. chris.smith-at-bbsrc.ac.uk
Most injuries while trimming blocks with hand-held razor blades result either from the free hand not knowing where the razor hand is, or from sudden uncontrolled movement of the blade when force is released at end of cut, or due to slippage, etc. when the razor hand / arm movement is unlimited. A couple of simple rules will prevent these situations from arising. 1) Look before you move 2) when cutting, use both hands - hold one end of the blade in each hand at all times. That way you know where both hands are in relation to the blade all the time and there is also improved control over blade movement 3) Never cut with the blade at the end of an unsupported arm. Arms and hands should be supported as close to the specimen as possible, so that blade movement is strictly limited to the range that can be driven by deliberate finger movements, and free, involuntary movements cannot occur.
I recommend you not to wear gloves because they interfere with touch perception and interfere with your grip on the blade. Has your safety officer seen you in action? Does he really know what the risks are, or is his imagination running riot? Show him your procedures. (Any gender-specificity in the above is wholly unintentional)
Chris Jeffree University of Edinburgh Biological Sciences EM Facility
} Hi Listers, } I've been thrown on the scrapheap at 60. So I'll be unsubscribing soon but } will keep an eye on the list over a colleague's shoulder. Many thanks for } all the help and interesting items, especially the forensic stuff - a } fascinating and useful insight into the problems of others. } Byeeee, Chris, Plant Path., IACR-Rothamsted, UK. chris.smith-at-bbsrc.ac.uk
Chris -
WRONG attitude! I retired at the same age, and started Project MICRO so that I could continue to share my love of the microworld. I suggest that you contact the RMS equivalent, AMFES, and have some fun yourself!
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
Dear Listers, Many thanks indeed for the unanticipated response to my 'for info' note. Attitude adjustment assimilated. The world will hear from me again! ttfn, Chris
Still looking...for a few good account representatives for an electron and optical microscopy service. territory is open., excellent earning potential. Please call Dick O'Connellat 734-668-3309 or e-mail Oconnell-at-ltu.edu. for more information. (I was unable to reach some of you who responded because of one reason or another--you know who you are. Please contact me again with a phone number or some other means to reach you.)
We are looking for someone with EDS/SEM experience to work out of our Florida office. Responsible for setting up procedures and repairing systems in house as well as customer sites. Working without supervision is a must. if you are interested to know more about the position, please send your qualification and salary history to our Email address. rangets-at-aol.com
Dear Colleage, Does anybody know if there is a software that can create the atomic structure for an interface or a dislocation, so that an image simulation (by using EMS or Mac Tempas) can be carried out directly for such structures? I know crystal Kit can create an interface structure,however, its atomic cordinations can not be exported directly to MacTempas or EMS directly for image simulations.
I would be greatly appreciate if you could provide such kind of information!
Sincerely,
James
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Hello, I a trying to stain sections of plant root that has been infected with a fungus to highlight certain features including lignin, callose, suberin and the fungal tissue itself. However, my samples have been embedded in LR White and Spurr's Resins. I am having difficulty finding protocols for staining of these resins. Most protocols refer to paraffin sections and it is not possible to use ethanol based stains for these resin sections. Does anyone know of any good references, books etc where I can find protocols for staining of these resins for LM? Thanks for your help. Rose
Several stains are used with resin embedded sections. The favorite seems to be Toluidine blue. This topic was discussed last March and several postings will be in the Archives. The differentiation method I contributed then, but to make this posting useful, I'll give here "my" complete method. There are many variants, most recently contributors to the histoserver were "frothing" how wonderful the results of staining with a combination of urea and Toluidine blue are - I have no experience with that.
Make up 0.5% Toluidine blue and 1% Borax in water. This will keep "forever" in a stoppered bottle on the bench. Keep with it a small funnel and a double layer filter paper.
Sections should be well adhering to a slide after heating on a 60-80 degree hotplate for some minutes after the sections had dried. Run a thick felt-tip pen around the section - on the underside. This will help locating sections and will not wash off.
Poor about 5ml of stain into the filter and apply a couple of drops to the sections. Sit the funnel back on the bottle recovering the stain.
Place the section on a hotplate and leave until the edge of the stain has dried up.
Now a few drops of water could be added to gently remove the remaining stain. This would result in a fairly intense, but blue-only staining.
Its better to differentiate. This is one of the most attractive features of the Toluidine stain as it can give a two colour, pink and blue rendition. This shows cell features similar to a double staining with Haematoxylin & Eosin.
After staining on a hotplate add a drop of acid alcohol and then rinse the slide with distilled water. The acid alcohol can destain partially or even completely, but a brief application brings forth the two colours.
Make acid alcohol by adding to 25ml of 50% Ethanol a couple of drops of 1N HCl. Cheers Jim Darley ProSciTech Microscopy PLUS PO Box 111, Thuringowa QLD 4817 Australia Ph +61 7 4774 0370 Fax:+61 7 4789 2313 service-at-proscitech.com Great microscopy catalogue, 500 Links, MSDS, User Notes ABN: 99 724 136 560 www.proscitech.com
On Tuesday, January 16, 2001 1:59 PM, Rosalie Daniel [SMTP:rosalie-at-deakin.edu.au] wrote: } } Hello, } I a trying to stain sections of plant root that has been infected with a } fungus to highlight certain features including lignin, callose, suberin and } the fungal tissue itself. However, my samples have been embedded in LR } White and Spurr's Resins. I am having difficulty finding protocols for } staining of these resins. Most protocols refer to paraffin sections and it } is not possible to use ethanol based stains for these resin sections. Does } anyone know of any good references, books etc where I can find protocols } for staining of these resins for LM? } Thanks for your help. } Rose } }
LR White is a methacrylate, and most routine paraffin stains can be used directly with minor time modifications (the methacrylate can give some background staining, but usually umimportant). Spurr's (and other epoxies) can also be stained with differential methods--primarily using Toluidine Blue or methylene blue. Check out Hayat's book on staining (MA Hayat, "Stains and Cytochemical Methods", Plenum Press, 1993). He includes a broad range of stains, including PAS, basic fuchsin-toluidine blue (similar to H&E), Azure II-methylene blue-safranin O, H&E, and a thionin-acridine orange (specifically for plant tissues). Another good source of references would be to go to PubMed (http://www.ncbi.nlm.nih.gov/PubMed) and do a search for stains, then for resins or methacrylate, combine your searches, and use the original papers (I know there are a lot out there). BTW, most suppliers of stains (e.g. EM Sciences, Polysciences, Ted Pella, EB Sciences, Fullam, Ladd, ProSciTech,SPI, etc) will have protocols for using their stains on LR White and Spurr's--another good source for you. Hope this helps.
Roger C. Moretz, Ph.D. Dept of Toxicology Boehringer Ingelheim Pharmaceuticals, Inc.
I have no financial interest in any of the mentioned vendors/suppliers (and if I missed anyone--I apologize, it was purely a senior moment).
(On Tue, 16 Jan 2001 14:59:03 +1100, Rosalie Daniel 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, } I a trying to stain sections of plant root that has been infected with a } fungus to highlight certain features including lignin, callose, suberin and } the fungal tissue itself. However, my samples have been embedded in LR } White and Spurr's Resins. I am having difficulty finding protocols for } staining of these resins. Most protocols refer to paraffin sections and it } is not possible to use ethanol based stains for these resin sections. Does } anyone know of any good references, books etc where I can find protocols } for staining of these resins for LM? } Thanks for your help. } Rose } } }
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Hello, I work with radicle tips and I'm looking for an effective stain in order to reveal different cellular types such as xylem and/ or phloem, but I'm havin some problemsa in finding protocols. Can anybody help me? Thanks Carmen Martín
One of our students was worried and put labeling tape (sometimes referred to as "time tape") along the edge to be held (we normally break a double edge in half). We also have a very graphic cartoon drawn by our grad student depicting a severed finger complete with blood (he was getting frustrated with the EM students...)
Regarding the safety officers - teach *them* to section...
John P. Shields, PhD Center for Ultrastructural Research 151 Barrow Hall University of Georgia Athens, GA 30602 706-542-4080 FAX 706-542-4271 jshields-at-cb.uga.edu
Hi Linda, I worked with isolated ventricular cells many years ago, and as I remember, there was always some variablilty of staining intensities between cells that were processed in the same sample. We used cell that were isolated using enzymatic treatment in conjunction with shaking ( I believe that was pretty standard. This was in the early 1980's, work with Beatrice Wittenberg and Thomas Robinson). Cells that ended up in the same dish for study, and were fixed & processed together, took the stains differently. We also used Ruthenium Red to stain the glycocalyx as well as Alcian Blue, Safraninin O, phenylene diamine and a few other stains. You can look up the papers by Simionescu & Simionescu from the 1970's for examples. Caveoli can also be visualized with careful staining of silver-grey sections. You can also try bismuth instead of lead, but use it at 1/10 the recipe's strength and for a shorter time.
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
The Department of Biological Sciences at Chicago State University is looking for an experienced electron microscopy technologist. We teach a course in TEM in the fall and SEM in the spring. In the summer we have students from several programs who learn about EM and complete a simple research project. We work on research projects with undergraduates, graduate students, and
faculty. We have a really nice facility with JEOL 1200 STEM, JEOL 2100 SEM, and RMC ultramicrotomes with cryo. We have a beautiful campus that is very easy to get to as it is right at
several major freeways. Our website will give you more information: WWW.CSU.EDU/jbrown/EM
In our lab we have been sputter coating with gold since the dawn of time. This has essentially been the "traditional" metal we have used for coating our non-conductive samples. We have found that in some of our applications that the gold grain is to large and is causing us problems in visualizing some of the smaller structures (primarily in engineering samples) that we are interested in. We currently sputter our samples for 1 to 4 minutes with a current reading of 18 to 20 mA using an argon atmosphere in the coater. We are aware that chromium and/or osmium coating are preferential to gold sputtering, but those technologies are not available to us at this time. What I would like to know is: 1) What are the advantages of using something other than gold as the target material (eg. Gold palladium, platinum palladium, or just platinum)? 2) Are there other materials that will work besides these metals that would give us equal service for small grain and a stable coating? 3) Are there operating conditions we could try that would still give us good coating but reduce the grain size of the film material? Thanks for your help,
Mike
====================================== Michael D. Standing BYU Microscopy Lab 401 WIDB Brigham Young University Provo, UT 84602
Hello listers- I am looking for a supplier of bakelite ring forms 1 inch in diameter (outside). Would someone contact me with that information. I can't find anything on the web. I appreciate your help! Many Thanks, Sarah -- Sarah A.W. Lundberg Electron Microanalysis and Imaging Laboratory Department of Geoscience, UNLV 4505 S. Maryland Parkway Box 454010 Las Vegas, NV 89154-4010
Dear Michael, you dont say what resolution you need, but if you cut the current on your existing gold system down to 4-5mA for 3 min or so, you may see a considerable improvement in the 10-50,000X range.
Sally Stowe
Dr Sally Stowe Facility Coordinator, ANU EMU Box 475 Canberra ACT 2601 AUSTRALIA stowe-at-rsbs.anu.edu.au fax 61 (0)2 6125 3218 or 6125 8525 http://www.anu.edu.au/EMU
} } } "Michael D. Standing" {Michael_Standing-at-byu.edu} 01/17/01 07:37am } } } ------------------------------------------------------------------------ The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Dear Listers:
In our lab we have been sputter coating with gold since the dawn of time. This has essentially been the "traditional" metal we have used for coating our non-conductive samples. We have found that in some of our applications that the gold grain is to large and is causing us problems in visualizing some of the smaller structures (primarily in engineering samples) that we are interested in. We currently sputter our samples for 1 to 4 minutes with a current reading of 18 to 20 mA using an argon atmosphere in the coater. We are aware that chromium and/or osmium coating are preferential to gold sputtering, but those technologies are not available to us at this time. What I would like to know is: 1) What are the advantages of using something other than gold as the target material (eg. Gold palladium, platinum palladium, or just platinum)? 2) Are there other materials that will work besides these metals that would give us equal service for small grain and a stable coating? 3) Are there operating conditions we could try that would still give us good coating but reduce the grain size of the film material? Thanks for your help,
Mike
====================================== Michael D. Standing BYU Microscopy Lab 401 WIDB Brigham Young University Provo, UT 84602
Ah, once again invaluable information, Thank you John, Fred and Nestor too!! I tried all the suppliers I could think of, except Buehler of course!
-- Sarah A.W. Lundberg Electron Microanalysis and Imaging Laboratory Department of Geoscience, UNLV 4505 S. Maryland Parkway Box 454010 Las Vegas, NV 89154-4010
Hi All, Here's an LM-related question: A group here needs to look at samples stained with picrosirius red using polarizing optics. I have a microscope equipped with DIC, and realize that if we pull the Wollaston prisms, we might be able to see something, but I don't have a rotatable stage which would make it easier to align their samples relative to the polarized light. Do any of you out there in the New York City area have an appropriate microscope? Or any ideas? TIA, 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 at South Bay Technology offer such a product. They are available as our Part Number RFP100-10 and cost $5.25 for a package of 10. We have them in stock and can ship them out the same day you order them. I hope this helps.
David Henriks Vice President TEL: 800-728-2233 (toll free in the USA) South Bay Technology, Inc. +1-949-492-2600 1120 Via Callejon FAX: +1-949-492-1499 San Clemente, CA 92673 USA e-mail: henriks-at-southbaytech.com
} } } } } Please visit us at http://www.southbaytech.com { { { { {
Manufacturers of precision sample preparation equipment and supplies for metallography, crystallography and electron microscopy.
Message text written by Sarah Lundberg } ------------------------------------------------------------------------ The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Hello listers- I am looking for a supplier of bakelite ring forms 1 inch in diameter (outside). Would someone contact me with that information. I can't find anything on the web. I appreciate your help! Many Thanks, Sarah -- Sarah A.W. Lundberg Electron Microanalysis and Imaging Laboratory Department of Geoscience, UNLV 4505 S. Maryland Parkway Box 454010 Las Vegas, NV 89154-4010
Hi all, I am working with seeds of Ilex paraguariensis (the maté). The aim of my research is to describe the ultrastructure (TEM) of the endosperm and the imature embryo. The samples (small dissected pieces) were fixed in glutaraldehyde and formaldehyde solution in phosphate buffer, washed, transferred for osmium (2% in 0,8% K3FeCN6, 1:1), dehydrated in acetone (10, 30, 50, 70, 90, 90 ,100, 100, 30 min in each step) and included in 1:3, 1:1, 3:1 and two changes of pure Spurr resin (24 hour in each step with continuous agitation). However, the tissues are very poorly infiltrated (endosperm and embryo with holes and soft parts). The endosperm cells have a lot of proteins and lipids as storage substances. I think that I should use a special protocol for this plant tissues, but I want to maintain the osmium fixation (lipid preservation). I tried the LR White and Unicryl resins with worst results. Does anybody suggest some thing? Thank's.
Dr. Rinaldo Pires dos Santos Lab. of Plant Anatomy Dept. of Botany - UFRGS Brazil e-mail: rinaldop-at-uol.com.br
you will find a lot of information in "Histochemistry" by R.W. Horobin, Stuttgart, G. Fischer 1982.
A few years ago I did some staining of plant cuticles (lets assume cutin is similar to suberin for your purpose) with Sudan Black B in Epon sections. SBB needs to be dissolved in hot alcohol but it worked quiet well on my Epon semis. I even managed to dissolve the resin in KOH before staining and got good results ... A recipe for SBB staining you will find in Bronner, R., 1975: Simultanous Staining of Lipid and Starch in Plant Tissues. Stain Technology 50(1):1-4.
I do not know if you want to use Toluidin Blue O, but TBO is a water based stain for acid polyanions like pectins, DNA/RNA and stains cytoplasm too. It will stain paraffin and resin sections and is easy and relatively safe to use. A very basic paper describing it is: Sakai, S.W, 1973: Simple method for differential staining of paraffin embedded plant material using Toluidin Blue O. Stain Tech 48(5):247-249.
Hope that helps you,
Joachim
Dr. Joachim Prutsch Product Manager EM Specimen Preparation
------- Forwarded message follows ------- } From: Alexander Tikhonovski {tikhonov-at-mpi-halle.mpg.de} To: "Pier, Julie (LNA)" {Julie.Pier-at-america.luzenac.com}
Hi Rinaldo,
I have been working on the ultrastructure of orchid stigmas for a few years, this tissue contains a large amount of lipids and intercellular cutin, debris from plasmolysed "nutritive cells", slimy pectins etc ... very difficult to embed - at least that was what everbody told me when I started. As in the orchid column the pollen (pollinia in this case) is still there, in most cases I embedded even the pollen with its sporopollenin, a lipidic substance usually extremely bad to embed (sections may break out at the interface to the resin).
In the beginning I tried Spurr and had very poor results. Then I switched to Epon although everybody told me that this would work even worse because of the high viscosity of Epon (= bad infiltration).
But I could achieve godd embedding with Epon for my tissue. Here is how I did it:
Specimen: Orchid buds, columns and stigmas, preferably smaller then 2x2x2 mm Fixation: 3% GAD in cacodylate buffer pH7.2 for at least 24 h Wash a few times in buffer and then in a.d. Stepwise dehydration in acetone: 30, 50, 70, 90, 100, 100% for 20 min each Intermedium acetontril 3 x 100% for 10 min each Embedding in Epon (Agar 100 Resin Kit): No movement of the specimens needed, just use Eppendorf tubes or something similar acetonitril:Epon 3:1 overnight acetonitril:Epon 1:1 4 h acetonitril:Epon 1:3 4 h pure Epon overnight change to Epon + accelerator Polymerisation in flat embedding form 48 h at 60°C
I used the acetonitril as a substitute for propylene oxide simply because it is said to be less poisonous. Maybe its the acetonitril step that is responsible for the good infiltration - I really do not know, but it worked well, so "never change a winning team".
Hope that helps you,
Joachim
Dr. Joachim Prutsch Product Manager EM Specimen Preparation
15th International Congress on Electron Microscopy
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1 - 6 September 2002
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Mike, The obvious grains of Au are the reason that the Au/Pd alloy is used. It should be less apparent with a Au/Pd target. Ken Converse owner Quality Images Delta, PA
Michael D. Standing 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: } } In our lab we have been sputter coating with gold since the dawn of time. } This has essentially been the "traditional" metal we have used for coating } our non-conductive samples. We have found that in some of our applications } that the gold grain is to large and is causing us problems in visualizing } some of the smaller structures (primarily in engineering samples) that we } are interested in. We currently sputter our samples for 1 to 4 minutes with } a current reading of 18 to 20 mA using an argon atmosphere in the coater. } We are aware that chromium and/or osmium coating are preferential to gold } sputtering, but those technologies are not available to us at this time. } What I would like to know is: } 1) What are the advantages of using something other than gold as the target } material (eg. Gold palladium, platinum palladium, or just platinum)? } 2) Are there other materials that will work besides these metals that would } give us equal service for small grain and a stable coating? } 3) Are there operating conditions we could try that would still give us good } coating but reduce the grain size of the film material? } Thanks for your help, } } Mike } } ====================================== } Michael D. Standing } BYU Microscopy Lab } 401 WIDB } Brigham Young University } Provo, UT 84602 } } e-mail: Michael_Standing-at-byu.edu } phone: (801) 378-4011 } fax: (801) 378-3937 } ====================================== } } } } }
I would suggest you try gold/palladium. It has a smaller grain size and the same reflectivity.
John Arnott
Disclaimer: Ladd Research sell targets for most types of sputter coaters. --
LADD RESEARCH 131 Dorset Lane Williston, VT 05495 USA
web site http://www.laddresearch.com
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Michael D. Standing 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: } } In our lab we have been sputter coating with gold since the dawn of time. } This has essentially been the "traditional" metal we have used for coating } our non-conductive samples. We have found that in some of our applications } that the gold grain is to large and is causing us problems in visualizing } some of the smaller structures (primarily in engineering samples) that we } are interested in. We currently sputter our samples for 1 to 4 minutes with } a current reading of 18 to 20 mA using an argon atmosphere in the coater. } We are aware that chromium and/or osmium coating are preferential to gold } sputtering, but those technologies are not available to us at this time. } What I would like to know is: } 1) What are the advantages of using something other than gold as the target } material (eg. Gold palladium, platinum palladium, or just platinum)? } 2) Are there other materials that will work besides these metals that would } give us equal service for small grain and a stable coating? } 3) Are there operating conditions we could try that would still give us good } coating but reduce the grain size of the film material? } Thanks for your help, } } Mike } } ====================================== } Michael D. Standing } BYU Microscopy Lab } 401 WIDB } Brigham Young University } Provo, UT 84602 } } e-mail: Michael_Standing-at-byu.edu } phone: (801) 378-4011 } fax: (801) 378-3937 } ======================================
I have been doing cryoultramicrotomy for the last year or so with varying levels of success. I finally got some pretty pictures, so I know I can get it right. Now I want to make it consistent.
So, my biggest problem appears to be with freezing. I am fixing my cells with 4% para, 0.1% glut, 0.25M Hepes, rinsing with Hepes, embedding in 10% gelatin and then infiltrating with 2.3M sucrose in a stepwise manner. I am cutting the sample into *very* small blocks (less than 0.5mm) hoping to infiltrate better. I then place the sample onto pins and drop into liquid nitrogen to freeze. However, it always seems that only the very outer layer of tissue/cells are well frozen. If I take a 1 micron section to see how the tissue looks, I can't take another b/c it would bring me into a freeze damaged area. I have tried using liquid proprane and liquid freon, but the samples cracked when I attempted to section them.
I have now been given a very precious human sample that they want to immunolabel on cryo thin sections, and I don't have enough tissue to make lots of blocks to section just the outside.
If anyone has any suggestions to help me get good freezing deeper in the tissue, I'd appreciate it. TIA Leslie
These are my pretty pictures: http://www.aecom.yu.edu/aif/gallery/TEM/shields_immuno/tem_cryo.htm Analytical Imaging Facility visit our web site: www.aecom.yu.edu/aif Albert Einstein C. of M 1300 Morris Park Ave Forchheimer 639 Bronx, NY 10461 718-430-3547
It always amazes me how much discussion can be generated on some topics!
I very rarely offer my 'two cents', but love reading through the comments. On the issue of microtome safety: I have been an electron microscopist for over 25 years (I started as a child prodigy!) and other than one incident early on when I (stupidly) tried trimming a block by bringing the razor blade toward me, I have NEVER had a problem with severed fingers, major lacerations, etc.
The aforementioned incident did result in stitches and I bear the scar proudly.
I do my trimming on a special holder on the Reichert Ultracut looking through the binoculars and "map" out the block face by marking the edges with the blade. Then I proceed very carefully (away from me and the block) to trim the epon. I then do the rough sectioning on the microtome itself. At times, we have used a jeweler's saw and vise to trim away excess epon and get down to the tissue, etc.
I agree that gloves or other enhancements only add to the problem.
I believe the main thing to consider is: "Think before you cut!"
Peggy Sherwood -- Peggy Sherwood Lab Associate, Photopathology Wellman Laboratories of Photomedicine (W224) Massachusetts General Hospital 50 Blossom Street Boston, MA 02114 617-724-4839 (voice mail) 617-726-6983 (lab) 617-726-3192 (fax) sherwood-at-helix.mgh.harvard.edu
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