by sparc5.microscopy.com (8.9.3+Sun/8.9.3) with ESMTP id IAA00704 for {Microscopy-at-sparc5.Microscopy.Com} ; Wed, 1 May 2002 08:20:37 -0500 (CDT) Received: from utm-notesob1.mdacc.tmc.edu (utm-notesob1.mdacc.tmc.edu [143.111.88.29]) by mail.mdanderson.org (8.9.1b+Sun/8.9.1) with SMTP id IAA16901 for {Microscopy-at-MSA.Microscopy.Com} ; Wed, 1 May 2002 08:12:57 -0500 (CDT) Received: by utm-notesob1.mdacc.tmc.edu(Lotus SMTP MTA v4.6.7 (934.1 12-30-1999)) id 86256BAC.00486FB3 ; Wed, 1 May 2002 08:11:11 -0500 X-Lotus-FromDomain: MDACC To: Microscopy-at-sparc5.microscopy.com Message-ID: {86256BAC.00486A87.00-at-utm-notesob1.mdacc.tmc.edu}
Did you try Nikon? I have one that was was purchased from them about 10 years ago. The part number on it is 231262. ---------------------- Forwarded by Mannie Steglich/MDACC on 05/01/2002 08:15 AM ---------------------------
Susan Rehorek {susan.rehorek-at-sru.edu} on 04/30/2002 12:46:04 PM
To: Microscopy-at-sparc5.microscopy.com cc: (bcc: Mannie Steglich/MDACC)
I am looking for a Camera Lucida. This is a drawing tube + dissecting (stereo) microscope. I used these as an undergrad - and found them to be excellent for zone diagrams and gross pictures (photos give too much detail sometimes).
I have tried all the major vendors (in the US) I can think of.
Does anyone know where I can get these from? It doesn't have to be new, as long as it works.
Please reply off-list.
Thanks
Sue Susan J Rehorek, Ph.D. Department of Biology Slippery Rock University of Pennsylvania PA, 16057-1326
I have one. If you will contact me directly by email, we can make arrangements for what you need.
Mannie Steglich U T M D Anderson Cancer Center. ---------------------- Forwarded by Mannie Steglich/MDACC on 05/01/2002 08:22 AM ---------------------------
Margaret Miller {MILLERMM-at-uthscsa.edu} on 04/30/2002 10:33:01 AM
To: MSA: ; cc: (bcc: Mannie Steglich/MDACC)
-- Dear list, Does anyone have a service manual to the MT-2B Sorvall microtome. We are in need of a parts list. Thanks
Does anyone know of a mfg. that makes a camera, for general photography, that will accomodate 4x5" film like Polaroid Type 57, that uses a Graflok back? I checked with Polaroid but they could offer no assistance.
Thanks,
Peter Tomic Anadigics, Inc.
-----Original Message----- } From: Gary Gaugler [mailto:gary-at-gaugler.com] Sent: Tuesday, April 30, 2002 3:48 PM To: MSA listserver
There was a discussion thread here awhile ago about cut film holders for use instead of Polaroid materials. I have some 4x5" Riteway cut film holders for sale and a Horseman 120 roll film back, Mfr # 47022452. This roll film back fits Graflok backs found on most all SEMs. It works with any type of 120 roll film. The active image capture area is 6x7cm--so you won't get the normal field of view as that of a Polaroid or 4x5" cut film. But the film and processing is much cheaper than Polaroid.
The holders are $6ea and the roll back is $425 ($550 new). If no one is interested in these items, they will go to a photo selling venue.
It makes one wonder why anyone would post something on the Listserver & conceal their identity unless they had something to hide.
Then again, why would someone post an message like this unless they had something to gain or in revenge.
I havE neVer heard of rontec but assume that thEy are a X-ray company. For motivation, that lEaVes compEting X-ray Companies. HowEVer, I doubt that the largEr X-ray Companies would even bother. That leaves the smaller EDS Companies which would have equal motivation but would not see the repercussions of management.
I seem to vaguely recall a thread about a member evaluating EDS Companies & their service. Another member touted the superior service & capabilities of one of the EDS Companies in question. A colleague of mine questioned the identity of the second member & found that the second member had posted the message anonymously. When queried about their identity he got no response.
It would be interesting to identify this person.
I am not saying that there is a connection, just thinking out loud on the Listserver.
Earl Weltmer Scanservice Corporation My true identity ----- Original Message ----- } From: {zaluzec-at-sparc5.microscopy.com} To: {Microscopy-at-sparc5.microscopy.com} Cc: "Rontec Cust." {rtc998-at-toast.com} Sent: Tuesday, April 30, 2002 6:57 PM
I have a Philips CM12 TEM for sale. It was under service contract from Philips until about 3 years ago. It has not been used for over a year due to a vacuum leak in the column. All manuals and lots of spare parts are included, including the gaskets needed to repair the leak. Water recirculator is also included. The microscope is in central New Jersey. Best offer. Please contact me directly.
Geoff mcauliff-at-umdnj.edu -- ********************************************** Geoff McAuliffe, Ph.D. Neuroscience and Cell Biology Robert Wood Johnson Medical School 675 Hoes Lane, Piscataway, NJ 08854 voice: (732)-235-4583; fax: -4029 mcauliff-at-umdnj.edu **********************************************
Most, if not all, makes of 4x5 camera will accept Polaroid backs. I bought one years ago from Calumet Photo for about $200 (without lens!. The camera was a used Cambo 4x5, built like a tank.
Nikon makes a 35mm camera that will accept Polaroid film with the use of an expensive accessory, called a "magny", I believe. You could check with your local camera store on this, but a decent used 4x5 will certainly cost less.
Hope this helps.
Randy
Randy Tindall EM Specialist Electron Microscopy Core Facility W122 Veterinary Medicine University of Missouri Columbia, MO 65211 Tel: (573) 882-8304 Fax: (573) 884-5414 Email: tindallr-at-missouri.edu Web: http://www.biotech.missouri.edu/emc/
-----Original Message----- } From: Peter Tomic [mailto:PTomic-at-anadigics.com] Sent: Wednesday, May 01, 2002 8:45 AM To: MSA listserver
Folks;
Does anyone know of a mfg. that makes a camera, for general photography, that will accomodate 4x5" film like Polaroid Type 57, that uses a Graflok back? I checked with Polaroid but they could offer no assistance.
Thanks,
Peter Tomic Anadigics, Inc.
-----Original Message----- } From: Gary Gaugler [mailto:gary-at-gaugler.com] Sent: Tuesday, April 30, 2002 3:48 PM To: MSA listserver
There was a discussion thread here awhile ago about cut film holders for use instead of Polaroid materials. I have some 4x5" Riteway cut film holders for sale and a Horseman 120 roll film back, Mfr # 47022452. This roll film back fits Graflok backs found on most all SEMs. It works with any type of 120 roll film. The active image capture area is 6x7cm--so you won't get the normal field of view as that of a Polaroid or 4x5" cut film. But the film and processing is much cheaper than Polaroid.
The holders are $6ea and the roll back is $425 ($550 new). If no one is interested in these items, they will go to a photo selling venue.
I am trying to teach 4th graders how an oxygen saturation meter works, & my experiment is FAILING!! Basically, oxygen saturation is measured by passing 2 light beams through the finger, one red light (660 nm), the other infrared (940 nm). If the blood is oxygenated, it appears red because it absorbs red light, thus very little of the red beam passes through. If the blood has little oxygen, it appears blue & allows red light to pass. In both cases, the infrared beam will pass through. The amount of red vs infrared light detected on the other side of the finger is proportional to level of oxygen saturation.
I designed an experiment to show that a red laser pointer beam would be absorbed by red Kool-Aid, while blue Kool-Aid would allow the red beam to pass through. Unfortunately, this is not the case!!! The red Kool-Aid makes the laser beam darker if anything! PLEASE, can someone tell me what is going on? Is there any simple way to communicate this principle?? I appreciate your help.
Mary
*************************************************** Mary K.O'Connell Cardiovascular Biomechanics Research Lab MSLS: Room P224 - Surgery 1201 Welch Road Stanford, CA 94305 (650) 723-1695 (650) 498-6262 Fax E-mail: oconne1l-at-leland.stanford.edu (Note: O'Connell in the E-mail address is spelled with a numeric "1" for the first l, and an alphabetic "l" for the second.) *******************************************************
"Ginger Hendricks" To: "Doss, Phoebe and Mike" {pjdoss-at-okstate.edu} {grhendricks-at-cox. cc: (bcc: Phoebe J Doss/app/Cvm) net} Subject: please forward to the MSA listserv
05/01/02 04:13 PM
Hello all,
I have a researcher who is interested in using autoradiography with nerve tissue. His tech is researching methods and has come to me for advice. I have never performed this procedure and am concerned about sectioning "hot" (S35) tissue with the microtome. Any protocols, suggestions or direction would be greatly appreciated.
My email address is grhendricks-at-cox.net
Thank you in advance,
Ginger
Ginger R. Hendricks EM Lab Manager and Adjunct Instructor OSU-CHS 1111 W. 17th St. Tulsa, OK 74107 (918) 561-8232 work (918) 699-8629 fax grhendricks-at-cox.net Website: http://www.healthsciences.okstate.edu/research/rsp/electronmicroscopy/electron_microscopy_laboratory.htm
Hi there, Does anyone have a ballpark figure for the cost of a new tabletop automatic processor for black and white printing? Currently we use an Ilford 2150RC processor. We are thinking of switching to digital printing off negatives and are doing some costings. Thanks.
John Brealey, EM Unit, Queen Elizabeth Hospital, Adelaide, South Australia
As soon as it's in the plastic, it should not be a problem. S35 - is very moderate beta emitter, 26 cm of air/0.32 mm of water will completely block it. Half-life is 84 days - keep in mind: work faster than decay. Most important part is labelling and embedding. Check solutions for radionuclides after processing the sample with Geiger detector, dispose properly. Amount of radioactivity in sections is negligible: less or equal to uranyl-acetate staining. Hope it may help. Sergey
At 02:22 PM 5/1/02, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
_____________________________________
Sergey Ryazantsev Ph. D. Electron Microscopy UCLA School of Medicine Department of Biological Chemistry Box 951737 Los Angeles, CA 90095-1737
Raj, was the cryopump made by Balzers? If not, I suspect it was made by CTI Cryogenics - try www.ctivacuum.com for parts, service, or replacement. I don't know for sure if they have used/rebuilt - they may. Also try www.bidservice.com for used cryopumps and Helium compressors.
No interest in either one, just passing the information along.
Vitaly Feingold Scientific Instruments and Applications 2773 Heath Lane, Duluth GA 30096 (770)232-7785 ph. (770)232-1791 fax (678)467-0012 mobile
This message is made of 100% recycled electrons. ----- Original Message ----- } From: Raj Patel {rpatel-at-umdnj.edu} To: {microscopy-at-sparc5.microscopy.com} Sent: Wednesday, May 01, 2002 12:56 PM
Earl, try these:
1) Malin Co., 5400 Smith Road, Brook Park, OH 44142. Specialty wire. Tel. (216)267-9080. I don't know if they have a web site. 2) Alfa Aesar, www.alfa.com , (800)343-0660, and (800)343-7276 for tech support. 3) Little Falls Alloys, www.lfa-wire.com , (888)5329473 or (973)278-1666.
Alfa will probably have the purest Copper, as far as Oxygen and other impurities go (the best is 99,9999% metals basis). Little Falls Alloys may have more suitable specialty Copper alloy, especially for high temperature apps.
Vitaly Feingold Scientific Instruments and Applications 2773 Heath Lane, Duluth GA 30096 (770)232-7785 ph. (770)232-1791 fax (678)467-0012 mobile
This message is made of 100% recycled electrons. ----- Original Message ----- } From: Earl Weltmer (by way of MicroscopyListserver) {earlw-at-sbcglobal.net} To: {Microscopy-at-sparc5.microscopy.com} Sent: Wednesday, May 01, 2002 7:36 PM
Mary Isn't this backwards? Oxygenated blood appears redder in transmitted or reflected light because it absorbs *blue*, and transmits or reflects the remaining red. } Basically, oxygen saturation is measured by } passing 2 light beams through the finger, one red light (660 nm), the other } infrared (940 nm). If the blood is oxygenated, it appears red because it } absorbs red light, thus very little of the red beam passes through. If the } blood has little oxygen, it appears blue & allows red light to pass. In } both cases, the infrared beam will pass through. The amount of red vs } infrared light detected on the other side of the finger is proportional to } level of oxygen saturation.
Again I think you have this the wrong way round. Red Kool-Aid looks red because it allows red light to pass through. Think of the effect of shining a white torch beam through red KoolAid onto a sheet of white paper. What colour is the beam? Red. Why, because that is the predominant colour of light remaining in the beam, blue and green having been removed by the KoolAid. A Blue filter should attenuate a red laser more than a Red filter, assuming the two are of the same colour strength.
The only way the red KoolAid can absorb more red light than the blue is if it contains more red-absorbing (i.e. cyan or blue) dye than is present in the Blue KoolAid. This seems unlikely, but is not impossible. Which flavour do you use for red, and which for blue? The crimson effect of black cherry is almost certainly produced by combining red and blue dyes, and there may be more blue dye in black cherry than there is in ice-blue raspberry.
You might find the following web sites instructive
http://www.dartmouth.edu/~chemlab/chem6/dyes/full_text/chemistr y.html#dyestruct http://www.dartmouth.edu/~chemlab/info/resources/spectrum/spectr um.html Chris
} I designed an experiment to show that a red laser pointer beam would be } absorbed by red Kool-Aid, while blue Kool-Aid would allow the red beam to } pass through. Unfortunately, this is not the case!!! The red Kool-Aid makes } the laser beam darker if anything! PLEASE, can someone tell me what is } going on? Is there any simple way to communicate this principle?? I } appreciate your help. } } Mary } } *************************************************** } Mary K.O'Connell } Cardiovascular Biomechanics Research Lab } MSLS: Room P224 - Surgery } 1201 Welch Road } Stanford, CA 94305 } (650) 723-1695 } (650) 498-6262 Fax } E-mail: oconne1l-at-leland.stanford.edu } (Note: O'Connell in the E-mail address is spelled with a numeric "1" for } the first l, and an alphabetic "l" for the second.) } ******************************************************* }
========================================== Dr. Chris Jeffree University of Edinburgh BIOSEM - Biological Sciences Electron Microscope Facility Institute of Cell and Molecular Biology Waddington Building King's Buildings, Mayfield Road EDINBURGH, EH9 3JN, Scotland, UK Tel. #44 (0) 131 650 5554 FAX. #44 (0) 131 650 6563 Mobile 07710 585 401 email c.jeffree-at-ed.ac.uk =========================================
I think Chris is right. I got your message late last night and started to reply that plants are green because they reflect green light, then I in my sleepy state I started thinking that maybe something is different about reflected versus transmitted light and I gave up trying to help.
However, this morning I still think the red should pass through red Koolaid better than ultraviolet. I haven't had this stuff since my undergrad about 20 years ago.
Karen Pawlowski, Ph.D. UT Dallas
Chris Jeffree 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 } -----------------------------------------------------------------------. } } Mary } Isn't this backwards? Oxygenated blood appears redder in } transmitted or reflected light because it absorbs *blue*, and } transmits or reflects the remaining red. } } Basically, oxygen saturation is measured by } } passing 2 light beams through the finger, one red light (660 nm), the other } } infrared (940 nm). If the blood is oxygenated, it appears red because it } } absorbs red light, thus very little of the red beam passes through. If the } } blood has little oxygen, it appears blue & allows red light to pass. In } } both cases, the infrared beam will pass through. The amount of red vs } } infrared light detected on the other side of the finger is proportional to } } level of oxygen saturation. } } Again I think you have this the wrong way round. Red Kool-Aid } looks red because it allows red light to pass through. Think of the } effect of shining a white torch beam through red KoolAid onto a } sheet of white paper. What colour is the beam? Red. Why, } because that is the predominant colour of light remaining in the } beam, blue and green having been removed by the KoolAid. A Blue } filter should attenuate a red laser more than a Red filter, assuming } the two are of the same colour strength. } } The only way the red KoolAid can absorb more red light than the } blue is if it contains more red-absorbing (i.e. cyan or blue) dye than } is present in the Blue KoolAid. This seems unlikely, but is not } impossible. Which flavour do you use for red, and which for blue? } The crimson effect of black cherry is almost certainly produced by } combining red and blue dyes, and there may be more blue dye in } black cherry than there is in ice-blue raspberry. } } You might find the following web sites instructive } } http://www.dartmouth.edu/~chemlab/chem6/dyes/full_text/chemistr } y.html#dyestruct } http://www.dartmouth.edu/~chemlab/info/resources/spectrum/spectr } um.html } Chris } } } I designed an experiment to show that a red laser pointer beam would be } } absorbed by red Kool-Aid, while blue Kool-Aid would allow the red beam to } } pass through. Unfortunately, this is not the case!!! The red Kool-Aid makes } } the laser beam darker if anything! PLEASE, can someone tell me what is } } going on? Is there any simple way to communicate this principle?? I } } appreciate your help. } } } } Mary } } } } *************************************************** } } Mary K.O'Connell } } Cardiovascular Biomechanics Research Lab } } MSLS: Room P224 - Surgery } } 1201 Welch Road } } Stanford, CA 94305 } } (650) 723-1695 } } (650) 498-6262 Fax } } E-mail: oconne1l-at-leland.stanford.edu } } (Note: O'Connell in the E-mail address is spelled with a numeric "1" for } } the first l, and an alphabetic "l" for the second.) } } ******************************************************* } } } } ========================================== } Dr. Chris Jeffree } University of Edinburgh } BIOSEM - Biological Sciences Electron Microscope Facility } Institute of Cell and Molecular Biology } Waddington Building } King's Buildings, Mayfield Road } EDINBURGH, EH9 3JN, Scotland, UK } Tel. #44 (0) 131 650 5554 } FAX. #44 (0) 131 650 6563 } Mobile 07710 585 401 } email c.jeffree-at-ed.ac.uk } =========================================
we do microtomy/TEM of bacterial samples with U and Tc in our lab. We take special precautions at the block trimming part by collecting all the chips on a piece of tape and disposing of them, as well as of the unused sections, as a rad waste. I don't think my little routine of wiping the microtome after finishing the work helps anything but my consciousness, however, it may make you feel better, too. Since I am using a TEM that is NOT devoted to the rad work (I think that will be also your case), I make a duplicate grid, and run it through the scintillation counter. If the count doesn't exceed background (most of the cases - imagine the dimensions of a section), I consider it non rad. Your S35 beta should be a very safe bet. Please feel free to contact me if you need any more info, Alice.
Alice Dohnalkova Environmental Microbiology Pacific Northwest National Laboratory MS P7-50 Richland, WA 99352 tel. (509) 372-0692 office (509) 376-3654 TEM lab fax (509) 376-1321
} From: Phoebe J Doss/app/Cvm [SMTP:pjdoss-at-cvm.okstate.edu] Sent: Wednesday, May 01, 2002 2:23 PM To: microscopy-at-sparc5.microscopy.com
"Ginger
Hendricks" To: "Doss, Phoebe and Mike" {pjdoss-at-okstate.edu} {grhendricks-at-cox. cc: (bcc: Phoebe J Doss/app/Cvm) net} Subject: please forward to the MSA listserv
05/01/02 04:13 PM
Hello all,
I have a researcher who is interested in using autoradiography with nerve tissue. His tech is researching methods and has come to me for advice. I have never performed this procedure and am concerned about sectioning "hot" (S35) tissue with the microtome. Any protocols, suggestions or direction would be greatly appreciated.
My email address is grhendricks-at-cox.net
Thank you in advance,
Ginger
Ginger R. Hendricks EM Lab Manager and Adjunct Instructor OSU-CHS 1111 W. 17th St. Tulsa, OK 74107 (918) 561-8232 work (918) 699-8629 fax grhendricks-at-cox.net Website: http://www.healthsciences.okstate.edu/research/rsp/electronmicroscopy/electr on_microscopy_laboratory.htm
I suggest that you check out the following reference
Dickson, G.R., 1984; Chemical fixation and the preparation of calcified tissues for transmission electron microscopy in: G.R. Dickson (ed) Methods of Calcified Tissue Research. New York, Elsevier, pp 79-148
Bob Robert J. Schmitz Department of Biology University of Wisconsin Stevens Point Stevens Point, WI 54481 715-346-2420 Email: rschmitz-at-uwsp.edu http://biology.uwsp.edu/faculty/RSchmitz/home.html
} ---------- } From: Fernando Capela e Silva } Sent: Wednesday, April 24, 2002 5:20 PM } To: microscopy-at-sparc5.microscopy.com } Subject: SEM and TEM for bone } } ------------------------------------------------------------------------ } 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 would like someone send me a general bone preparation scheme for SEM and } TEM. } } With compliments } * * * * * * * * * * * * * * * * * * * * * * } Fernando Capela e Silva } Laboratório de Biologia da Conservaçăo } Departamento de Biologia } Universidade de Évora } Apartado 94 } 7002-554 Évora } PORTUGAL } } Phone: +351-266 760 800 } Fax: +351-266 711 231 } Email: fcs-at-uevora.pt } } http://evunix.uevora.pt/~fcs/FernandoCapelaSilva.htm } } }
Center for Advanced Material Department of Chemical Engineering University of Massachusetts, Lowell Xianglin_Li-at-student.uml.edu Tel: 978-934-3411
----- Original Message ----- } From: Michael Green {michael.green-at-UCL.AC.UK}
Hello all!! I have a quick question for everyone.....We have a Hitachi 7500 TEM. We have been having a problem with "grainy" negatives, I don't think the focus is as crisp as it should be. I have tried smaller apertures (both obj. and cond. in various combinations). If we take pictures of the same sample on a different microscope, the micrographs are not grainy and the focus is much clearer (so it's not the sample, the negatives, or the paper we're using....). I know the optical density setting for the camera can be changed to increase contrast, I have a feeling this would increase graininess as well...is my hunch correct? The kicker is that we have had the same optical density setting for weeks now and the graininess is just getting worse (to my knowledge nothing has changed on the microscope....). Would the use (or lack of use) of liquid Nitrogen influence graininess? Any other ideas or comments? Any help would be appreciated!!
Check out a Beldon Cable catalog. They sell different gauges of a good grade of Copper cable (unshielded/unwrapped). The copper conductor in the cables is probably a good grade also, but it may not be OFHC (Oxygen-free High Conductivity). I have no idea whether Beldon has their catalog on the web or not.
-Scott
Scott D. Walck, Ph.D. PPG Industries, Inc. Glass Technology Center P. O. Box 11472 (letters) Guys Run Rd. (packages) Pittsburgh, PA 15238-0472
Walck-at-PPG.com
(412) 820-8651 (office) (412) 820-8515 (fax)
-----Original Message----- } From: Vitaly Feingold [mailto:vitalylazar-at-worldnet.att.net] Sent: Thursday, May 02, 2002 2:47 AM To: Microscopy-at-sparc5.microscopy.com; Earl Weltmer (by way of MicroscopyListserver)
Earl, try these:
1) Malin Co., 5400 Smith Road, Brook Park, OH 44142. Specialty wire. Tel. (216)267-9080. I don't know if they have a web site. 2) Alfa Aesar, www.alfa.com , (800)343-0660, and (800)343-7276 for tech support. 3) Little Falls Alloys, www.lfa-wire.com , (888)5329473 or (973)278-1666.
Alfa will probably have the purest Copper, as far as Oxygen and other impurities go (the best is 99,9999% metals basis). Little Falls Alloys may have more suitable specialty Copper alloy, especially for high temperature apps.
Vitaly Feingold Scientific Instruments and Applications 2773 Heath Lane, Duluth GA 30096 (770)232-7785 ph. (770)232-1791 fax (678)467-0012 mobile
This message is made of 100% recycled electrons. ----- Original Message ----- } From: Earl Weltmer (by way of MicroscopyListserver) {earlw-at-sbcglobal.net} To: {Microscopy-at-sparc5.microscopy.com} Sent: Wednesday, May 01, 2002 7:36 PM
Heaven forbid that I should comment on something in the life science, so I won't. I don't think that Chris is correct in his explanation.
Let me site the example of a thin film of gold. If it is thin enough, when you look at the gold in transmission, it is green. In reflection it is gold because the gold is absorbing the green and allowing all other wavelengths of light to be reflected. If you make the gold thicker the intensity of the green getting through decreases exponentially with thickness until eventually it is opaque. A series of thickness of gold films from very thin to very thick illustrates the point very well.
I suspect that the absorption mechanism with the oxygen is related to the iron in the blood. Isn't it iron in the blood that carries the oxygen? With more oxygenated iron, a higher absorption occurs, i.e. the red light gets absorbed more. This is analogous to your beam getting darker. I would say that to show a less oxygenated example, you have to dilute your Cool-Aid.
-Scott
Scott D. Walck, Ph.D. PPG Industries, Inc. Glass Technology Center P. O. Box 11472 (letters) Guys Run Rd. (packages) Pittsburgh, PA 15238-0472
Walck-at-PPG.com
(412) 820-8651 (office) (412) 820-8515 (fax)
-----Original Message----- } From: Chris Jeffree [mailto:cjeffree-at-srv0.bio.ed.ac.uk] Sent: Thursday, May 02, 2002 6:45 AM To: Mary K. O'Connell Cc: microscopy-at-sparc5.microscopy.com
Mary Isn't this backwards? Oxygenated blood appears redder in transmitted or reflected light because it absorbs *blue*, and transmits or reflects the remaining red. } Basically, oxygen saturation is measured by } passing 2 light beams through the finger, one red light (660 nm), the other } infrared (940 nm). If the blood is oxygenated, it appears red because it } absorbs red light, thus very little of the red beam passes through. If the } blood has little oxygen, it appears blue & allows red light to pass. In } both cases, the infrared beam will pass through. The amount of red vs } infrared light detected on the other side of the finger is proportional to } level of oxygen saturation.
Again I think you have this the wrong way round. Red Kool-Aid looks red because it allows red light to pass through. Think of the effect of shining a white torch beam through red KoolAid onto a sheet of white paper. What colour is the beam? Red. Why, because that is the predominant colour of light remaining in the beam, blue and green having been removed by the KoolAid. A Blue filter should attenuate a red laser more than a Red filter, assuming the two are of the same colour strength.
The only way the red KoolAid can absorb more red light than the blue is if it contains more red-absorbing (i.e. cyan or blue) dye than is present in the Blue KoolAid. This seems unlikely, but is not impossible. Which flavour do you use for red, and which for blue? The crimson effect of black cherry is almost certainly produced by combining red and blue dyes, and there may be more blue dye in black cherry than there is in ice-blue raspberry.
You might find the following web sites instructive
http://www.dartmouth.edu/~chemlab/chem6/dyes/full_text/chemistr y.html#dyestruct http://www.dartmouth.edu/~chemlab/info/resources/spectrum/spectr um.html Chris
} I designed an experiment to show that a red laser pointer beam would be } absorbed by red Kool-Aid, while blue Kool-Aid would allow the red beam to } pass through. Unfortunately, this is not the case!!! The red Kool-Aid makes } the laser beam darker if anything! PLEASE, can someone tell me what is } going on? Is there any simple way to communicate this principle?? I } appreciate your help. } } Mary } } *************************************************** } Mary K.O'Connell } Cardiovascular Biomechanics Research Lab } MSLS: Room P224 - Surgery } 1201 Welch Road } Stanford, CA 94305 } (650) 723-1695 } (650) 498-6262 Fax } E-mail: oconne1l-at-leland.stanford.edu } (Note: O'Connell in the E-mail address is spelled with a numeric "1" for } the first l, and an alphabetic "l" for the second.) } ******************************************************* }
========================================== Dr. Chris Jeffree University of Edinburgh BIOSEM - Biological Sciences Electron Microscope Facility Institute of Cell and Molecular Biology Waddington Building King's Buildings, Mayfield Road EDINBURGH, EH9 3JN, Scotland, UK Tel. #44 (0) 131 650 5554 FAX. #44 (0) 131 650 6563 Mobile 07710 585 401 email c.jeffree-at-ed.ac.uk =========================================
Yeeess!, but haemoglobin is not reflective like gold. The gold phenomenon is caused by strong forward reflection of red/yellow light, and transmission of remaining green. Blood cells have no surface reflectivity to speak of. Blood is more like an emulsion of a red transparent phase in a pale yellow transparent phase. The oxygenated rbcs absorb blue, transmitting red, but they also cause light scattering, and some red light is forward scattered as a result. Unlike a film of gold, blood is red in reflected and transmitted light.
Now how do you explain the fact that colloidal gold appears red against the light i.e. red is transmitted?? Chris
p.s. you're allowed - we're talking physics here } Heaven forbid that I should comment on something in the life science, so I won't. I don't think that Chris is correct in his explanation. } } Let me site the example of a thin film of gold. If it is thin enough, when you look at the gold in transmission, it is green. In reflection it is gold because the gold is absorbing the green and allowing all other wavelengths of light to be reflected. If you make the gold thicker the intensity of the green getting through decreases exponentially with thickness until eventually it is opaque. A series of thickness of gold films from very thin to very thick illustrates the point very well. } } I suspect that the absorption mechanism with the oxygen is related to the iron in the blood. Isn't it iron in the blood that carries the oxygen? With more oxygenated iron, a higher absorption occurs, i.e. the red light gets absorbed more. This is analogous to your beam getting darker. I would say that to show a less oxygenated example, you have to dilute your Cool-Aid. } } -Scott } } Scott D. Walck, Ph.D. } PPG Industries, Inc. } Glass Technology Center } P. O. Box 11472 (letters) } Guys Run Rd. (packages) } Pittsburgh, PA 15238-0472 } } Walck-at-PPG.com } } (412) 820-8651 (office) } (412) 820-8515 (fax) } } } } -----Original Message----- } From: Chris Jeffree [mailto:cjeffree-at-srv0.bio.ed.ac.uk] } Sent: Thursday, May 02, 2002 6:45 AM } To: Mary K. O'Connell } Cc: microscopy-at-sparc5.microscopy.com } Subject: Re: Basic Science - oxygen saturation example } } } -------------------------------------------------------------------- ---- } 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 } -------------------------------------------------------------------- ---. } } } Mary } Isn't this backwards? Oxygenated blood appears redder in } transmitted or reflected light because it absorbs *blue*, and } transmits or reflects the remaining red. } } Basically, oxygen saturation is measured by } } passing 2 light beams through the finger, one red light (660 nm), the other } } infrared (940 nm). If the blood is oxygenated, it appears red because it } } absorbs red light, thus very little of the red beam passes through. If the } } blood has little oxygen, it appears blue & allows red light to pass. In } } both cases, the infrared beam will pass through. The amount of red vs } } infrared light detected on the other side of the finger is proportional to } } level of oxygen saturation. } } Again I think you have this the wrong way round. Red Kool-Aid } looks red because it allows red light to pass through. Think of the } effect of shining a white torch beam through red KoolAid onto a } sheet of white paper. What colour is the beam? Red. Why, } because that is the predominant colour of light remaining in the } beam, blue and green having been removed by the KoolAid. A Blue } filter should attenuate a red laser more than a Red filter, assuming } the two are of the same colour strength. } } The only way the red KoolAid can absorb more red light than the } blue is if it contains more red-absorbing (i.e. cyan or blue) dye than } is present in the Blue KoolAid. This seems unlikely, but is not } impossible. Which flavour do you use for red, and which for blue? } The crimson effect of black cherry is almost certainly produced by } combining red and blue dyes, and there may be more blue dye in } black cherry than there is in ice-blue raspberry. } } You might find the following web sites instructive } } http://www.dartmouth.edu/~chemlab/chem6/dyes/full_text/chemistr } y.html#dyestruct } http://www.dartmouth.edu/~chemlab/info/resources/spectrum/spectr } um.html } Chris } } } I designed an experiment to show that a red laser pointer beam would be } } absorbed by red Kool-Aid, while blue Kool-Aid would allow the red beam to } } pass through. Unfortunately, this is not the case!!! The red Kool-Aid makes } } the laser beam darker if anything! PLEASE, can someone tell me what is } } going on? Is there any simple way to communicate this principle?? I } } appreciate your help. } } } } Mary } } } } *************************************************** } } Mary K.O'Connell } } Cardiovascular Biomechanics Research Lab } } MSLS: Room P224 - Surgery } } 1201 Welch Road } } Stanford, CA 94305 } } (650) 723-1695 } } (650) 498-6262 Fax } } E-mail: oconne1l-at-leland.stanford.edu } } (Note: O'Connell in the E-mail address is spelled with a numeric "1" for } } the first l, and an alphabetic "l" for the second.) } } ******************************************************* } } } } } ========================================== } Dr. Chris Jeffree } University of Edinburgh } BIOSEM - Biological Sciences Electron Microscope Facility } Institute of Cell and Molecular Biology } Waddington Building } King's Buildings, Mayfield Road } EDINBURGH, EH9 3JN, Scotland, UK } Tel. #44 (0) 131 650 5554 } FAX. #44 (0) 131 650 6563 } Mobile 07710 585 401 } email c.jeffree-at-ed.ac.uk } =========================================
I don't want to make this more complicated as it is, but do you know, how Koolaid gets its color?
Could be straight exitation and relaxation. Then Koolaid would absorb a photon and emit it again. Since the emission should be into 4 Pi solid angle, the effect would be, that fewer photons of that color reach the eye, i.e., this color would be absorbed.
Could be a "fluorescence" effect, where Koolaid absorbs a high energy photon (blue), then emits a red photon and an IR photon. In this case the red parts of the spectrum would be enhanced.
Could be scattering, as in "why is the sky blue".
And then, the laser frequency may not be the one that is actually absorbed by Koolaid. Red is not necesarily red.
I think, without knowing exactly what it is that makes Koolaid red it is hard to predict what happens. And if that then can be applied to the color of blood is another step.
It might be easier to start with something different than Koolaid.
} } } } } } } } } } WE HAVE MOVED { { { { { { { { { please make a note of the new address below
Michael Bode, Ph.D. Soft Imaging System Corp. 12596 West Bayaud Avenue Suite 300 Lakewood, CO 80228 =================================== phone: (888) FIND SIS (303) 234-9270 fax: (303) 234-9271 email: mailto:info-at-soft-imaging.com web: http://www.soft-imaging.com ===================================
-----Original Message----- } From: Karen Pawlowski [mailto:kpawlow-at-swbell.net] Sent: Thursday, May 02, 2002 7:59 AM To: MSA listserver submission
Mary,
I think Chris is right. I got your message late last night and started to reply that plants are green because they reflect green light, then I in my sleepy state I started thinking that maybe something is different about reflected versus transmitted light and I gave up trying to help.
However, this morning I still think the red should pass through red Koolaid better than ultraviolet. I haven't had this stuff since my undergrad about 20 years ago.
Karen Pawlowski, Ph.D. UT Dallas
Chris Jeffree 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 } -----------------------------------------------------------------------. } } Mary } Isn't this backwards? Oxygenated blood appears redder in } transmitted or reflected light because it absorbs *blue*, and } transmits or reflects the remaining red. } } Basically, oxygen saturation is measured by } } passing 2 light beams through the finger, one red light (660 nm), the other } } infrared (940 nm). If the blood is oxygenated, it appears red because it } } absorbs red light, thus very little of the red beam passes through. If the } } blood has little oxygen, it appears blue & allows red light to pass. In } } both cases, the infrared beam will pass through. The amount of red vs } } infrared light detected on the other side of the finger is proportional to } } level of oxygen saturation. } } Again I think you have this the wrong way round. Red Kool-Aid } looks red because it allows red light to pass through. Think of the } effect of shining a white torch beam through red KoolAid onto a } sheet of white paper. What colour is the beam? Red. Why, } because that is the predominant colour of light remaining in the } beam, blue and green having been removed by the KoolAid. A Blue } filter should attenuate a red laser more than a Red filter, assuming } the two are of the same colour strength. } } The only way the red KoolAid can absorb more red light than the } blue is if it contains more red-absorbing (i.e. cyan or blue) dye than } is present in the Blue KoolAid. This seems unlikely, but is not } impossible. Which flavour do you use for red, and which for blue? } The crimson effect of black cherry is almost certainly produced by } combining red and blue dyes, and there may be more blue dye in } black cherry than there is in ice-blue raspberry. } } You might find the following web sites instructive } } http://www.dartmouth.edu/~chemlab/chem6/dyes/full_text/chemistr } y.html#dyestruct } http://www.dartmouth.edu/~chemlab/info/resources/spectrum/spectr } um.html } Chris } } } I designed an experiment to show that a red laser pointer beam would be } } absorbed by red Kool-Aid, while blue Kool-Aid would allow the red beam to } } pass through. Unfortunately, this is not the case!!! The red Kool-Aid makes } } the laser beam darker if anything! PLEASE, can someone tell me what is } } going on? Is there any simple way to communicate this principle?? I } } appreciate your help. } } } } Mary } } } } *************************************************** } } Mary K.O'Connell } } Cardiovascular Biomechanics Research Lab } } MSLS: Room P224 - Surgery } } 1201 Welch Road } } Stanford, CA 94305 } } (650) 723-1695 } } (650) 498-6262 Fax } } E-mail: oconne1l-at-leland.stanford.edu } } (Note: O'Connell in the E-mail address is spelled with a numeric "1" for } } the first l, and an alphabetic "l" for the second.) } } ******************************************************* } } } } ========================================== } Dr. Chris Jeffree } University of Edinburgh } BIOSEM - Biological Sciences Electron Microscope Facility } Institute of Cell and Molecular Biology } Waddington Building } King's Buildings, Mayfield Road } EDINBURGH, EH9 3JN, Scotland, UK } Tel. #44 (0) 131 650 5554 } FAX. #44 (0) 131 650 6563 } Mobile 07710 585 401 } email c.jeffree-at-ed.ac.uk } =========================================
If it's focus problem, try to make 'focus series' - the same area with 1,2,3 clicks to the left and to the right. You have to see the changes on the negs (and on the screen). I usually align microscope in the way that I am able to see changes from underfocus to overfocus in 3 clicks (it's JEM1200EX, coarse control) at x60-80K. So, 1st click is underfocus, next- focus, next - overfocus. If you do not see it, you have, probably, problem with alignment. I don't know how this related to your particular problem. In biological applications we are usually using amplitude contrast, so it's close to the actual focus. At this point you have minimal visual contrast. From that you defocus (to increase contrast and 'granularity' will go up too) your image. The degree of defocus depends what you want to see.
Personally, I would suspect film/developer/technician. So many things: bad batch of the film, film stored at the high temp, contaminated developer, unproper dilution etc. Try to make blank image (no sample in the microscope), turn off automatic exposure and make a few shots with different exposure time (around automatic measurements, say automatic is 2 sec, make 1, 1.5, 2, 3 sec) and develop altogether....
Sergey
At 12:56 PM 5/2/02, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
_____________________________________
Sergey Ryazantsev Ph. D. Electron Microscopy UCLA School of Medicine Department of Biological Chemistry Box 951737 Los Angeles, CA 90095-1737
We have stained annelid embryos with FITC-conjugated anti-tubulin antibody and propidium iodide. We are using a Biorad-MRC-600 and seem to be getting almost identical signals(of nuclei and a few mitochondria) on both the 488 and 568 wavelengths, even though when viewed with epifluorescence, the tubulin stain seems to distinctly define cell borders. I understood that the propidium iodide emission would not be overlapping with that of FITC--is this incorrect? I have other double-labelled samples which are stained with different stains, but their signals are within the appropriate emission spectra for both confocal and epifluorescence, so the detection filters on the confocal do not seem to be the problem.
I was considering purchasing a Kodak MDS 100 Digital camera to permanently attach to one of my microscopes for examining specimens directly on my computer CRT. Unfortunately as far as I can determine the software supplied only supports Win 95 and 98. I'd like to know if anyone is currently using a MDS 100 on ME or XP and how (or if) it works. Thanks in advance P Polsgrove
Pete Polsgrove NAU Flagstaff, AZ. pjp6-at-dana.ucc.nau.edu micro2001p-at-netscape.net
Karli, do grainy negatives look denser? If so, they may be overexposed (TEM setting/exp.meter problem), or overdeveloped (developer/temperature/time/stop bath). I assume here that the batch of film is fine. If grainy negatives don't look denser, then the problem is likely with TEM. It's difficult to say whether you are dealing with real photo emulsion grain, or rather with sample/TEM artifact, without seeing the negative.
Speaking of the emulsion grain- it will also appear on the normal density negatives, in the following cases: film improperly stored or expired, negatives were overexposed and underdeveloped or vice versa, in order to keep density normal. Then, bad developer (contaminated/exhausted), or bad film.
Use Sergey's advice and take a few blanks. It's hard to imagine a TEM problem causing that, other than incorrect exposure meter reading.
Vitaly Feingold Scientific Instruments and Applications 2773 Heath Lane, Duluth GA 30096 (770)232-7785 ph. (770)232-1791 fax (678)467-0012 mobile
This message is made of 100% recycled electrons. ----- Original Message ----- } From: Karli Fitzelle (by way of MicroscopyListserver) {fitzelle.1-at-osu.edu} To: {Microscopy-at-sparc5.microscopy.com} Sent: Thursday, May 02, 2002 3:56 PM
Mary, As someone who has used a pulse oximeter before a double lung transplant, I decided to dig out my manual. I am copying the following FYI:
"The pulse oximeter shines red and infrared light through the tissue and detects the fluctuating signals caused by arterial blood pulses. The ratio of the fluctuations of the red and infrared light signals received determines the oxygen saturation content. Conditions such as steady venous blood flow, skin thickness, finger nail thickness, etc. do not effect the saturation reading because they are constant and do not cause fluctuations."
(the function is then given as a formula; it goes on saying)
"Note that the oximeter's readings do not depend upon the absolute light intensity, rather upon the fluctuations in light intensity."
It goes on with other comments about skin pigmentation, if there is too little light, etc.
"Pulse oximeters use two different wavelengths of light (red and infrared), providing the ability to determine one component of the blood. The oximeter is calibrated to closely approximate functional oxygen saturation values. These values will closely approximate laboratory instrument functional saturation values if the dysfunctional hemoglobin saturation levels are negligible. If the dysfunctional hemoglobin is carboxyhemoglobin or methemoglobin, the difference between the oxygen saturation value displayed by the oximeter and the oxygen saturation values determined by the laboratory instrument will be greater as the dysfunctional hemoglobin levels rise approximately in accordance with the following formula: " (it then gives the formula).
I wonder if the issue is not "red blood" but how the red and infrared light interact with oxygenated and deoxygenated hemoglobin and not what we see as arterial (red) blood or venous (blue) blood. I don't think that this is an easy principle for 4th graders.
Chris gives a correct explanation about light absorption and the dyes used in Kool-Aid.
PS I hope this is part of a "Don't smoke" program!!!
Damian
Damian Neuberger, PhD Senior Research Scientist Baxter Healthcare Corp P.O. Box 490 Round Lake, IL 60073 Tel: 847.270.5888 Fax: 847.270.5897 damian_neuberger-at-baxter.com
} Need Your Help!! } } I am trying to teach 4th graders how an oxygen saturation meter works, & my } experiment is FAILING!! Basically, oxygen saturation is measured by } passing 2 light beams through the finger, one red light (660 nm), the other } infrared (940 nm). If the blood is oxygenated, it appears red because it } absorbs red light, thus very little of the red beam passes through. If the } blood has little oxygen, it appears blue & allows red light to pass. In } both cases, the infrared beam will pass through. The amount of red vs } infrared light detected on the other side of the finger is proportional to } level of oxygen saturation. } } I designed an experiment to show that a red laser pointer beam would be } absorbed by red Kool-Aid, while blue Kool-Aid would allow the red beam to } pass through. Unfortunately, this is not the case!!! The red Kool-Aid makes } the laser beam darker if anything! PLEASE, can someone tell me what is } going on? Is there any simple way to communicate this principle?? I } appreciate your help. } } Mary } } *************************************************** } Mary K.O'Connell } Cardiovascular Biomechanics Research Lab } MSLS: Room P224 - Surgery } 1201 Welch Road } Stanford, CA 94305 } (650) 723-1695 } (650) 498-6262 Fax } E-mail: oconne1l-at-leland.stanford.edu } (Note: O'Connell in the E-mail address is spelled with a numeric "1" for } the first l, and an alphabetic "l" for the second.) } ******************************************************* } }
Check with Calumet Photographic. Their web address is
www.calumetphoto.com
Damian Neuberger
} Folks; } } Does anyone know of a mfg. that makes a camera, for general photography, } that will accomodate 4x5" film like Polaroid Type 57, that uses a Graflok } back? I checked with Polaroid but they could offer no assistance. } } Thanks, } } Peter Tomic } Anadigics, Inc.
Talking about ultra-fine gold foil or gold colloidal suspension, we have to keep in mind the'wave-nature' of the light. When thickness of material is comparable to wavelength, so may magical things is happening: suspended tiny gold particles colored solution in the red. Moreover, the color depends from the particle size - you could make it brownish or greenish - depends how much tannic acid you add to make collodial gold. Over moreover: you could calculate the particles size from the known spectrum. Similar things is happening with fine gold foil. I was a bad student in the physic class. I do remember it's waves. If particle is smaller than 1/2 wavelength, the wave will not interfere with it. Red light has longer wavelength and pass gold particles when other has adsorbed. I hope it's how they teach us... Sorry if I am wrong. Similar to lasers. It's monochromatic and coherent. To filter it you should use appropriate things: diffraction (pattern?) filters (they work similarly: let pass wavelength longer then the size of the strips). If KoolAid is looks red it does not mean it will be transparent to the laser wavelength. I think the set of simple photographic filters (red/blue; yellow/green) may do better job (I mean, no lasers).
Sergey
At 02:43 PM 5/2/02, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
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Sergey Ryazantsev Ph. D. Electron Microscopy UCLA School of Medicine Department of Biological Chemistry Box 951737 Los Angeles, CA 90095-1737
{bold} {color} {param} 0100,0100,0100 {/param} To the Microscopy & Microanalysi= s community
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Hi folks - I'm familar with prep for TEM, SEM, etc., but not confocal - would you send me a good protocol for this type of scope for tissue or single cells? Thanks Barb
Hi folks - I'm familar with prep for TEM, SEM, flow, etc., but not this type of scope, would someone send me a good protocol for tissue and single cells? Thanks Barb
Yes, they do reflect green light. But they also transmit green light. Chlorophylls a and b have two strong absorption peaks very roughly between 400&500nm and between 650 and 700nm. The remaining central part of the visible spectrum appears green, but also contains cyan, yellow and orange.
} I think Chris is right. I got your message late last night and started } to reply that plants are green because they reflect green light, then I } in my sleepy state I started thinking that maybe something is different } about reflected versus transmitted light and I gave up trying to help. } } However, this morning I still think the red should pass through red } Koolaid better than ultraviolet. I haven't had this stuff since my } undergrad about 20 years ago. } } Karen Pawlowski, Ph.D. } UT Dallas } } Chris Jeffree 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 } } -----------------------------------------------------------------------. } } } } Mary } } Isn't this backwards? Oxygenated blood appears redder in } } transmitted or reflected light because it absorbs *blue*, and } } transmits or reflects the remaining red. } } } Basically, oxygen saturation is measured by } } } passing 2 light beams through the finger, one red light (660 nm), the other } } } infrared (940 nm). If the blood is oxygenated, it appears red because it } } } absorbs red light, thus very little of the red beam passes through. If the } } } blood has little oxygen, it appears blue & allows red light to pass. In } } } both cases, the infrared beam will pass through. The amount of red vs } } } infrared light detected on the other side of the finger is proportional to } } } level of oxygen saturation. } } } } Again I think you have this the wrong way round. Red Kool-Aid } } looks red because it allows red light to pass through. Think of the } } effect of shining a white torch beam through red KoolAid onto a } } sheet of white paper. What colour is the beam? Red. Why, } } because that is the predominant colour of light remaining in the } } beam, blue and green having been removed by the KoolAid. A Blue } } filter should attenuate a red laser more than a Red filter, assuming } } the two are of the same colour strength. } } } } The only way the red KoolAid can absorb more red light than the } } blue is if it contains more red-absorbing (i.e. cyan or blue) dye than } } is present in the Blue KoolAid. This seems unlikely, but is not } } impossible. Which flavour do you use for red, and which for blue? } } The crimson effect of black cherry is almost certainly produced by } } combining red and blue dyes, and there may be more blue dye in } } black cherry than there is in ice-blue raspberry. } } } } You might find the following web sites instructive } } } } http://www.dartmouth.edu/~chemlab/chem6/dyes/full_text/chemistr } } y.html#dyestruct } } http://www.dartmouth.edu/~chemlab/info/resources/spectrum/spectr } } um.html } } Chris } } } } } I designed an experiment to show that a red laser pointer beam would be } } } absorbed by red Kool-Aid, while blue Kool-Aid would allow the red beam to } } } pass through. Unfortunately, this is not the case!!! The red Kool-Aid makes } } } the laser beam darker if anything! PLEASE, can someone tell me what is } } } going on? Is there any simple way to communicate this principle?? I } } } appreciate your help. } } } } } } Mary } } } } } } *************************************************** } } } Mary K.O'Connell } } } Cardiovascular Biomechanics Research Lab } } } MSLS: Room P224 - Surgery } } } 1201 Welch Road } } } Stanford, CA 94305 } } } (650) 723-1695 } } } (650) 498-6262 Fax } } } E-mail: oconne1l-at-leland.stanford.edu } } } (Note: O'Connell in the E-mail address is spelled with a numeric "1" for } } } the first l, and an alphabetic "l" for the second.) } } } ******************************************************* } } } } } } } ========================================== } } Dr. Chris Jeffree } } University of Edinburgh } } BIOSEM - Biological Sciences Electron Microscope Facility } } Institute of Cell and Molecular Biology } } Waddington Building } } King's Buildings, Mayfield Road } } EDINBURGH, EH9 3JN, Scotland, UK } } Tel. #44 (0) 131 650 5554 } } FAX. #44 (0) 131 650 6563 } } Mobile 07710 585 401 } } email c.jeffree-at-ed.ac.uk } } ========================================= } }
========================================== Dr. Chris Jeffree University of Edinburgh BIOSEM - Biological Sciences Electron Microscope Facility Institute of Cell and Molecular Biology Waddington Building King's Buildings, Mayfield Road EDINBURGH, EH9 3JN, Scotland, UK Tel. #44 (0) 131 650 5554 FAX. #44 (0) 131 650 6563 Mobile 07710 585 401 email c.jeffree-at-ed.ac.uk =========================================
Every time I have had a really excessive grain problem it was from using too strong a concentration of developer, way too strong or I was underexposing the film and over developing it. The first was usualy by accident and only caused a problem when I was working with a completely unknown set of conditions such as infra red photography, a new film and a mistake in dilution where I had to establish exposure time, development time without reliable tools to measure the intensity of the infra red light or working with some new combination of film and some unconventional developer. I the last case it was usualy intentionally trying to take pictures in light to low for the film I had.
Gordon
} From: "Sergey Ryazantsev" {sryazant-at-ucla.edu} : Karli : : If it's focus problem, try to make 'focus series' - the same area with : 1,2,3 clicks to the left and to the right. You have to see the changes on : the negs (and on the screen). I usually align microscope in the way that I : am able to see changes from underfocus to overfocus in 3 clicks (it's : JEM1200EX, coarse control) at x60-80K. So, 1st click is underfocus, next- : focus, next - overfocus. If you do not see it, you have, probably, problem : with alignment. I don't know how this related to your particular : problem. In biological applications we are usually using amplitude : contrast, so it's close to the actual focus. At this point you have : minimal visual contrast. From that you defocus (to increase contrast and : 'granularity' will go up too) your image. The degree of defocus depends : what you want to see. : : Personally, I would suspect film/developer/technician. So many things: bad : batch of the film, film stored at the high temp, contaminated developer, : unproper dilution etc. Try to make blank image (no sample in the : microscope), turn off automatic exposure and make a few shots with : different exposure time (around automatic measurements, say automatic is 2 : sec, make 1, 1.5, 2, 3 sec) and develop altogether.... : : Sergey : : At 12:56 PM 5/2/02, you wrote: : } ------------------------------------------------------------------------ : } The Microscopy ListServer -- Sponsor: The Microscopy Society of America : } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com : } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html : } -----------------------------------------------------------------------. : } : } : } Hello all!! : } I have a quick question for everyone.....We have a Hitachi 7500 : } TEM. We have been having a problem with "grainy" negatives, I don't think : } the focus is as crisp as it should be. I have tried smaller apertures : } (both obj. and cond. in various combinations). If we take pictures of the : } same sample on a different microscope, the micrographs are not grainy and : } the focus is much clearer (so it's not the sample, the negatives, or the : } paper we're using....). I know the optical density setting for the camera : } can be changed to increase contrast, I have a feeling this would increase : } graininess as well...is my hunch correct? The kicker is that we have had : } the same optical density setting for weeks now and the graininess is just : } getting worse (to my knowledge nothing has changed on the : } microscope....). Would the use (or lack of use) of liquid Nitrogen : } influence graininess? Any other ideas or comments? : } Any help would be appreciated!! : } : } Thanks, : } : } Karli : : _____________________________________ : : Sergey Ryazantsev Ph. D. : Electron Microscopy : UCLA School of Medicine : Department of Biological Chemistry : Box 951737 : Los Angeles, CA 90095-1737 : : Phone: (310) 825-1144 : FAX (departmental): (310) 206-5272 : mailto:sryazant-at-ucla.edu : : : : :
It's strange to see that one anonymous message could make so much damage to the company. It seems to me that reputation of the company depends more on the quality of the products/service etc nor on the one anonymous opinion. From another hand, I think, this ListServer mostly is a place for 'customers' to exchange not only scientific ideas but to help each other to survive in this 'capitalistic' world. Information about wrongdoing may help others do not make similar mistake or spend money on bad quality product/service. This is sort of our 'protection' against bad quality service/products providers. Again, single decision even published here could not damage the reputation of the good company with long well established record of the service to EM community. I know, there are places on the Internet where you could leave your opinion about some particular business/company - it's perfectly legal and many institutions used that lists for decision making. This discussion is more about ethics - we all agree that we have rights openly speak here and others have the rights to know who is speaking.
Sergey spoke.
At 02:15 AM 5/3/02, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
_____________________________________
Sergey Ryazantsev Ph. D. Electron Microscopy UCLA School of Medicine Department of Biological Chemistry Box 951737 Los Angeles, CA 90095-1737
To get a better sense of this thread of conversation I went looking for a source of concentration on this specific subject. This continued an attempt some time ago when the question came up on another 'List'.
As we learn from one another, sometimes it helps to find a source of expertise who appears to have actually been involved in the engineering of the type of device in question - or something like it. Further, the following URL demonstrates that this conversation is ALL about physics
Thus, I recommend some outside reading at: http://lfd.uiuc.edu/staff/maier/thesis/index.html
Is it widely known that some arctic fish travel contentedly sans RBCs? For more information look in old 'Comparative Biochemistry' by Baldwin. Short book from Methuen and a longer one from Cambridge. Also a reading from Sci. Am.: http://oak.cats.ohiou.edu/~piccard/scientam/globins.html
Also, HIGHLY recommended is the translation of Zinoffsky's original paper on hemoglobin: http://www.udel.edu/chem/white/teaching/CHEM342/ZinBkgd99.html
For me life is just a constant stream of history and future, mixed in the present. As George Patton said (about something else!), "God help me, I do love it so."
Regards,
Fred Monson
P.S. Award for best Commencement Address ever goes to Kurt Vonnegut (1997 -at- MIT) even if he didn't give it: http://www.tiac.net/users/sqltech/document/vonegut.txt
Frederick C. Monson, PhD Center for Advanced Scientific Imaging Schmucker II Science Center West Chester University South Church Street and Rosedale West Chester, Pennsylvania, USA, 19383 Phone: 610-738-0437 FAX: 610-738-0437 fmonson-at-wcupa.edu CASI URL: http://darwin.wcupa.edu/casi/ WCUPA URL: http://www.wcupa.edu/ Visitors URL: http://www.wcupa.edu/_visitors/
} ---------- } From: Mary K. O'Connell } Sent: Wednesday, May 1, 2002 4:45 PM } To: Microscopy-at-sparc5.microscopy.com } Subject: Basic Science - oxygen saturation example } } ------------------------------------------------------------------------ } 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 } -----------------------------------------------------------------------. } } } Need Your Help!! } } I am trying to teach 4th graders how an oxygen saturation meter works, & } my } experiment is FAILING!! Basically, oxygen saturation is measured by } passing 2 light beams through the finger, one red light (660 nm), the } other } infrared (940 nm). If the blood is oxygenated, it appears red because it } absorbs red light, thus very little of the red beam passes through. If the } } blood has little oxygen, it appears blue & allows red light to pass. In } both cases, the infrared beam will pass through. The amount of red vs } infrared light detected on the other side of the finger is proportional to } } level of oxygen saturation. } } I designed an experiment to show that a red laser pointer beam would be } absorbed by red Kool-Aid, while blue Kool-Aid would allow the red beam to } pass through. Unfortunately, this is not the case!!! The red Kool-Aid } makes } the laser beam darker if anything! PLEASE, can someone tell me what is } going on? Is there any simple way to communicate this principle?? I } appreciate your help. } } Mary } } *************************************************** } Mary K.O'Connell } Cardiovascular Biomechanics Research Lab } MSLS: Room P224 - Surgery } 1201 Welch Road } Stanford, CA 94305 } (650) 723-1695 } (650) 498-6262 Fax } E-mail: oconne1l-at-leland.stanford.edu } (Note: O'Connell in the E-mail address is spelled with a numeric "1" for } the first l, and an alphabetic "l" for the second.) } ******************************************************* } }
At 09:37 PM 5/2/2002 -0500, Damian Neuberger wrote: } I wonder if the issue is not "red blood" but how the red and infrared light } interact with oxygenated and deoxygenated hemoglobin and not what we see as } arterial (red) blood or venous (blue) blood. I don't think that this is an } easy principle for 4th graders.
Yes, half of them will come away thinking that red Kool-Aid has blood in it. :-) The good news is that 20% of them weren't paying attention and won't retain this "fact".
I need to do flat embedding using LR White. A Teflon mold covered with ACLAR seems to be the answer. I am afraid that the over filled resin under ACLAR may not polimerize properly and become messy. I appreciate your experience.
Hi All: I am trying to convert an image and spectra from the Oxford AN 10000 EDS to a .tiff that is readable on a PC. I've done it in the past, but it has been so long, I forget the exact procedure. I hope that there is somone out there that does this more regularly that can refresh my memory. Thanks in advance, Mike Coviello UT Arlington
The following TEM, which is capable of producing images with 0.17 nm resolution, but has gun/filament instability problems especially above 300 KV, is available to anyone willing to take responsibility for removing it from its present location prior to August 2002. There is no charge other than the costs involved with dismantling, moving, shipping and reinstallation. It is a top-entry version of a JEOL 4000. The only accessory is a Gatan image intensifier and TV camera. It is estimated that it would take two weeks to dismantle and pack properly for reuse. It is located in Ithaca, NY at Cornell University's Center for Materials Research.
} Try food coloring. Tried it. Didn't like it. Fact is green potatoes and bright purple steak just doesn't get eaten.
The take-home from this discussion, as pointed out by several respondents, is that there are several ways to arrive at "red" in Kool-Aid, inkjet inks, food colouring, whatever. For example, a red which exactly matches the apparent colour of a laser pointer could be produced by a single red dye, or, as in an inkjet printer, from a blend of yellow and magenta dyes. A deeper cherry red from your printer will be a blend of yellow, magenta and cyan dyes. What is required is some data on the absorption/transmission characteristics of different reds and blues. The best thing would be to run an absorption spectrum using a spectrophotometer. If there is no chance of access to one then it might be instructive to do some simple chromatography. Place drops of concentrated solutions of fibre-tip pen, fabric dye, food colouring or Kool-Aid one inch from the long edge of a ~12" x 6" piece of filter paper or blotting paper. Curl the paper into a cylinder, holding the short edges together with a staple or paper clip and stand (the paper!) in 3/8" of water in a suitable lidded container. 15-20 minutes later you will have a colourful chromatographic separation of the main dyes in your samples. Get the kids involved - they'll love it.
The First International Conference on Biomedical Spectroscopy: } From Molecules to Men 7-10 July, 2002 Cardiff, Wales, United Kingdom
This conference covers spectroscopic as well as application of microscopic techniques, such as AFM, for analysis of biological/biomedical systems.
Information regarding the conference is given below. You can also visit the web-site of the conference:
http://www.dmu.ac.uk/In/biospectra/
Best wishes, Dr P.I. Haris Editor-in-chief: Spectroscopy - An International Journal Editor: Biochemical Journal Department of Biological Sciences, De Montfort University, The Gateway, Leicester, LE1 9BH, United Kingdom E-Mail: pharis-at-dmu.ac.uk
First International Conference on Biomedical Spectroscopy: } From Molecules to Men 7-10 July, 2002 Cardiff, Wales, United Kingdom
Aims and Scope of the Conference:
The first international conference on Biomedical Spectroscopy will bring together spectroscopists and life scientists, from academia and industry, engaged in solving problems of biological and biomedical interest using diverse spectroscopic techniques. The conference is dedicated to the memory of Professor Dennis Chapman FRS who introduced many spectroscopic techniques to the study of biological systems. The interdisciplinary nature of the conference will encourage scientific interchange and cross-fertilisation of ideas.
Application of spectroscopic techniques such as Mass spectrometry, CD, FTIR, NMR, EPR, ENDOR, NIR, SPR, Raman, EXAFS, UV/Visible, Atomic Force Spectroscopy, Neutron Spectroscopy, Dielectric Spectroscopy, Fluorescence Spectroscopy and so on, for solving problems in diverse areas of life science including -Biomedical and Clinical Science -Biochemistry and Biophysics -Biomaterials and Biosensors -Proteomics and Pharmaceuticals -Biotechnology and Biomedical Engineering
Call for Papers:
Scientists employing spectroscopic techniques in any area of life science research are invited to submit proposals for lectures and poster presentations. Papers presented at the conference will be reviewed and published in a special issue of Spectroscopy - An International journal (http://www.iospress.nl/site/navfr/navframe2.html)
Programme Structure:
The scientific programme will consist of invited lectures, as well as contributed lectures selected from submitted contributions. There will also be poster periods and time allocated for exhibition where participants can discuss with spectroscopic manufacturers.
Deadlines:
Early Registration: 31 May 2002 Abstract Submission: 15 June 2002 Manuscript Submission for Publication in Spectroscopy: 8 July 2002
Conference Organising Committee Members :
Jose Luis Arrondo (University Pais Vasco, Spain) Yoshinori Asakawa (Tokushima Bunri University, Japan) Laurence D, Barron, (University of Glasgow, UK) Andreas Barth (Johann Wolfgang Goethe Universitaet, Germany) Lawrence J. Berliner (University of Denver, USA) William Bonfield (University of Cambridge, UK) Kevin M. Brindle (University of Cambridge, UK) Chris Cooper (University of Essex, UK) Gerard Cote (Texas A&M University, USA) Lesley Davenport (CUNY, USA) Martyn C Davies (University of Nottingham, UK) Michael J. Davies (Heart Research Institute, Australia) Peter J. Derrick (University of Warwick, UK) David Gadian (Institute of Child Health, UK) Parvez I. Haris (De Montfort University, UK) Marcus A. Hemminga (Wageningen University, The Netherlands) Larry Hench (Imperial College, London, UK) Jan Johansson (Karolinska Institute, Stockholm, Sweden) Mikio Kataoka (Nara Institute of Science & Technology, Japan) Katrin Kneipp (Massachusetts Institute of Technology, USA) Wlfgang Knoll (Max-Planck-Institut für Polymerforschung, Germany) Kunihiro Kuwajima (University of Tokyo, Japan) James M. McDonnell (University of Oxford, UK) Henry H. Mantsch (Institute for Biodiagnostics, Canada) Jeremy Nicholson (Imperial College, London, UK) Niels Chr. Nielsen (University of Aarhus, Denmark) Eric Oldfield (University of Illinois, USA) Yukihiro Ozaki (Kwansei-Gakuin University, USA) Hazime Saito (Himeji Institute of Technology, Japan) Zhifeng Shao (University of Virginia School of Medicine, USA) Gary Siuzdak (The Scripps Research Institute, USA) Thomas G. Spiro (Princeton University, USA) Gordon Tollin (University of Arizona, USA) Bonnie Wallace (University of London, UK)
Conference Chair:
Dr P.I. Haris Editor-in-Chief: Spectroscopy - An International Journal http://www.iospress.nl/site/html/07124813.html Editor: Biochemical Journal http://www.biochemj.org/bj/bjedboard.htm Editorial Advisor: Molecular Membrane Biology http://www.tandf.co.uk/journals/boards/tmmb-edbrd.html Treasurer: Protein and Peptide Science Group of Biochemical Society & RSC http://www.biochemistry.org/groups/ppsg/members.htm
Further information regarding the conference should be addressed to:
Dr Parvez I. Haris Department of Biological Sciences, De Montfort University, The Gateway, Leicester, LE1 9BH, United Kingdom E-Mail: pharis-at-dmu.ac.uk Tel. 00-44-116-2506306 Fax: 00-44-116-2577287
REGISTRATION FORM:
Please send completed form by e-mail (pharis-at-dmu.ac.uk) to the Conference Chair or by regular post: Dr P.I. Haris, Department of Biological Sciences, De Montfort University, The Gateway, Leicester, LE1
Amount ..........Early Registration. Payment received before 31 May 2002 (Ł400) ..........Late Registration. Payment received after 31 May 2002: (Ł500) ..........Student (Ł300) ..........Accompanying Person (Ł250)* ..........Total amount
Registration fee covers the following: Accommodation for three nights in single rooms Conference dinner Lunch, tea, coffee for the duration of the conference Conference bag, as well as the Abstract and Programme Book. *Accompanying person registration fee covers accommodation for three nights, conference dinner, lunch, tea and coffee.
PAYMENTS:
Registration fee can be directly paid by bank transfer: transfer should be made to: 'Biospectra' Account, Account Number 02786668, Sort Code: 30-94-97, Lloyds TSB Bank, Leicester High Street Banch, Leicester, LE1 9FS, UK. The payments must be made in Sterling Pounds. Please state your name and address.
Alternatively the registration fee can be paid by cheque or international money order in Sterling Pounds, made payable to 'Biospectra'. The cheque should be sent by registered mail to Dr P.I. Haris, Department of Biological Sciences, De Montfort University, The Gateway, Leicester, LE1 9BH, United Kingdom.
Please send your payments by one of the above methods as soon as possible. After receipt of your payment e-mail conformation will be forwarded.
Accommodation:
Costs associated with accommodation are included within the registration fee. Accommodation will be in single rooms for three nights covering 7-10 July 2002. Anyone requiring accommodation for additional nights should contact the conference organiser in advance.
Information Regarding Arrival/Departure:
Date of arrival ........ / .......... / 2002 Date of departure ........ / .......... / 2002 *Need to be met at Cardiff Central Station: Yes/No *Need to be met at Cardiff International Airport: Yes/No
*Please indicate time of arrival at the station or the airport by e-mail.
Abstract Submission:
Any person registered to attend the conference may submit one Abstract where he/she is the main author. It is possible submit additional Abstracts where he/she is not the main author. The Organising committee will select some of the Abstracts for oral presentation. Please indicate if you are willing to present an oral presentation, if selected.
The Abstract must be on one page, be single spaced and fit into an A4 size portrait-oriented rectangular space. Times New Roman fonts should be used throughout the entire text of the abstract, including the title and author sections. The name of the author who will present the paper at the congress should be underlined. The Abstract should be prepared in MS WORD for Windows. Abstracts should be sent by e-mail to pharis-at-dmu.ac.uk or by regular post to the following address: Dr P.I. Haris, Department of Biological Sciences, De Montfort University, The Gateway, Leicester, LE1 9BH, United Kingdom. Fax: 00-44-116-2577287
Conference Publication:
Papers presented at the conference will be published in a special issue of Spectroscopy - An International Journal. Manuscripts should be submitted to the organisers at the Conference in Cardiff. Although there are no specific length restrictions, papers should be of a length appropriate to the material presented at the Conference. All papers will be reviewed and are expected to be of a standard expected for a paper published by the Journal in a regular issue.
The manuscripts should be prepared according to the instructions available at http://www.iospress.nl/site/html/07124813_ita.html The manuscript should be submitted at the conference in a diskette containing the electronic version of the manuscript, together with two paper copies.
The deadline for submission of manuscripts for publication in Spectroscopy - An International Journal is 8 July 2002.
Exhibition:
Space will be reserved for exhibition of diverse spectroscopic instrumentation, software, accessories, scientific journals and related books. Companies interested in participating should take immediate contact with the conference office.
Transportation:
Please let us know your travel plans so appropriate arrangements can be made to meet you in either Cardiff Central Station or at Cardiff International Airport.
London Heathrow Airport:
London's Heathrow Airport is the recommended route of arrival by air into the UK. From here you can travel directly to Cardiff by National Express coach (approximately 3 hours 15 minutes) or take the Heathrow Express (15 minutes) to London's Paddington station and catch a First Great Western The train journey to Cardiff Central station takes approximately 2 hours. Members of the organising committee will be available to meet the particpants at the Cardiff Central station. Please indicate your arrival plans in advance.
London Gatwick Airport:
You can travel to Cardiff directly by National Express coach (approximately 4 hours 45 minutes). Alternatively, you can take the Gatwick Express train to London's Victoria Station (30 minutes) and transfer to Victoria coach station from which the journey time is approximately 3 hours 10 minutes. Alternatively from Victoria, use the underground "Circle" line to reach Paddington Station and continue by train as above.
London Stansted and London Luton Airports:
Budget flights are available from Europe into these airports which both have rail and coach services into central London. For more information on travel options visit the Stansted and Luton airport websites.
Cardiff International Airport:
Cardiff International Airport which is situated 12 miles west of the city centre in Rhoose. Its main international connections are via Amsterdam (KLM), Brussels and Paris (British Airways). British Airways flights from Aberdeen, Edinburgh and Glasgow also serve the airport, as well as Ryanair and British Airways flights from Dublin. Members of the organising committee will be available to meet particpants arriving at the airport. Please indicate your arrival plans in advance.
Eurostar/Train:
Arrival by Eurostar is to London Waterloo station. There is a direct Great Western Train service from London Waterloo to Cardiff Central Station with an approximate journey of 3 hours 10 minutes. Alternatively, you may transfer at Waterloo to the underground "Bakerloo" line to London Paddington where you can take the train as above or take a coach from the Victoria station. Members of the organising committee will be available to meet particpants arriving at the Cardiff Central Station. Please indicate your arrival plans in advance.
Information about Cardiff and Wales:
You can find out more details about Wales from various guides including the Welsh Tourist Board (http://www.visitwales.com).
Cardiff, the capital city of Wales, boasts a number of tourist attractions and has an extensive shopping centre. The civic centre provides an interesting walking tour with many classical buildings including Cardiff City Hall. Nearby are Cardiff Castle and the Millennium Stadium. The National Museum (http://www.nmgw.ac.uk/) and Gallery is also very popular with visitors. There are many eating and drinking establishments situated in the city centre, ensuring that there is something for everyone. Virtual Cardiff (http://www.virtualcardiff.co.uk/) provides an indication of the wide variety entertainment taking place in the city. Cardiff Bay, a regenerated dock area, is a pleasant place to stroll around and can be reached by a short train journey or 30 minutes walk from Cardiff City centre. Cardiff, the Capital city is a lively, interesting and safe city.
Further afield:
There are many interesting attractions in South Wales attractions details of which can be found in various web-sites including Welsh Tourist Board (http://www.visitwales.com). and Data Wales (http://www.data-wales.co.uk/).
Activities:
Wales provides a wide variety of activities details of which can be found in a number of websites including the Welsh Tourist Board (http://www.visitwales.com). and Data Wales (http://www.data-wales.co.uk/)
Useful Links:
Information regarding Wales: http://www.visitwales.com Information Regarding Wales: http://www.data-wales.co.uk/ For UK train time tables visit www.railtrack.com To book UK rail tickets outside the UK visit www.britcities.com To book UK coach tickets visit www.gobycoach.com
Climate and Other Facts:
As Wales has a "temperate" climate, it generally never gets very hot or very cold. July should be one of the sunniest and warmest months of the year. However, it is advisable to bring a light rainproof coat and a sweater, just in case, but you might possibly be in T-shirts. If you are venturing into the mountains you will certainly need warmer clothing. You can get a better idea nearer the time from the UK Meteorological office (http://www.meto.gov.uk/).
Unfortunately that is the case. Someone posts damaging material on this (or any other) list, it get's sent around to some people a few times, and suddenly it is "the official opinion of the microscopy specialists". I am sure that can do substantial damage.
And it's not limited to the web or list servers. Audi (the German car manufacturer) had a good business going in the US until someone decided to start the engine and put it in forward (or backwards, I don't remember) and run the car into a wall. There was a flaw, that allowed users to put the car in gear without stepping on the brakes. Although that definitely was a flaw, it was blown out of proportion and almost killed the Audi business in the US. It took them 10 years to get their reputation back, even though I would not consider this as dangerous as the tire problem that Firestone/Ford was experiencing last year.
Bottom line: Everybody should be careful and check their sources when posting potentially dmaging material on the listserver.
But that's just my 2 cents as a vendor.
mike
} } } } } } } } } } WE HAVE MOVED { { { { { { { { { please make a note of the new address below
Michael Bode, Ph.D. Soft Imaging System Corp. 12596 West Bayaud Avenue Suite 300 Lakewood, CO 80228 =================================== phone: (888) FIND SIS (303) 234-9270 fax: (303) 234-9271 email: mailto:info-at-soft-imaging.com web: http://www.soft-imaging.com ===================================
-----Original Message----- } From: Sergey Ryazantsev [mailto:sryazant-at-ucla.edu] Sent: Friday, May 03, 2002 6:40 AM To: Microscopy-at-sparc5.microscopy.com
It's strange to see that one anonymous message could make so much damage to the company. It seems to me that reputation of the company depends more on the quality of the products/service etc nor on the one anonymous opinion. From another hand, I think, this ListServer mostly is a place for 'customers' to exchange not only scientific ideas but to help each other to survive in this 'capitalistic' world. Information about wrongdoing may help others do not make similar mistake or spend money on bad quality product/service. This is sort of our 'protection' against bad quality service/products providers. Again, single decision even published here could not damage the reputation of the good company with long well established record of the service to EM community. I know, there are places on the Internet where you could leave your opinion about some particular business/company - it's perfectly legal and many institutions used that lists for decision making. This discussion is more about ethics - we all agree that we have rights openly speak here and others have the rights to know who is speaking.
Sergey spoke.
At 02:15 AM 5/3/02, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
_____________________________________
Sergey Ryazantsev Ph. D. Electron Microscopy UCLA School of Medicine Department of Biological Chemistry Box 951737 Los Angeles, CA 90095-1737
Obviously, one can only conclude that the person(s) who sent this email are competitors of RÖNTEC.
I am the owner of a small business & have always been in favor of fair competition which benefits everyone. Occasionally, we have someone resort to "badmouthing" us in order sway an order. I have never felt it necessary as we have always had an abundance of business: relying on technical superiority & great customer relations.
I have found that equipment and Companies usually reflects the "personality" of the people involved. The same traits that I attribute to equipment (reliable, stable, solid) reflects the personality of the people. If the truth be known, I wonder about the integrity & reliability of equipment the "anonymous Sender" may market. It is obvious that he cannot sell based upon the equipment's technical merits.
It is ashamed that a member of this Listserver would find it necessary to resort to this "low-life" tactics. I wonder if the anonymous Sender can look with pride at his accomplishments & really take pride in himself for this feat.
My real name & my real Company for twenty years,
Earl Weltmer Scanservice Corporation ----- Original Message ----- } From: Thomas Schülein To: Microscopy-at-sparc5.microscopy.com Sent: Friday, May 03, 2002 2:15 AM
Hello microscopists, I am looking for a tried and true protocol for mouse bone. We are interested in looking at the osteoblasts, and I am not sure how to preserve them for examination of ultrathin sections in the TEM. What is the best decalcification method? What type of resin for embedding? Would a low viscosity resin, such as Spurr's, be the best? I would appreciate any help you could give. Thanks, Jo Dee Fish
************************************************************ Jo Dee Fish Research Technologist II Microscopy Core Gladstone Institute of Cardiovascular Disease
They were not totally anonymous since they had a real(?) email address. A posting inquiry to that address did not generate any response. So your point is well taken.
On a few occasions I have been handed reports from outside our organization with EDX spectra that were saved as image files, e.g. .bmp. .tif, .jpg etc. and pasted into a Word document or another report format. However, this "cut and paste job" is only an image and in my mind isn't data at all but simply information that can't be verified or refuted. A case in point is when I received a spectra that only displayed energies up to 3.5 KeV and the report identified Pt as Au which overlap at the lower energy region but spread out higher up. Now without the raw data I cannot do anything but take someone's word or politely interrogate the person that did the analysis. My question is whether it would be appropriate to ask someone on this listserver with the same EDX system to look at the raw data, if available, provided they have the same platform?
These matters are generally not life and death like a forensics issue but purely economic, but I'd rather be in jail than lose money.
The task of sharing spectra cross-platform was address a number of years ago by the MSA/MAS Standards Committee.
You could ask the individual to send the raw data to you in the MSA/MAS File format. You can then look at it on any computer with something as simple as a spread sheet program. In addition, a number of commerical manufacturers have implemented a routine to read/write data to/from this format, hence you might be able to look at the raw data on your own system.
You can find the details on the MSA/MAS format for Spectra at
======================== Keywords :XEDS,EELS,AES,WDS,CLS,GAM,XRF,PES Computer :IBM, MAC, DEC Operating System :ALL Programming Language :Fortran 77 Hardware Requirements :None Author(s) :EMSA/MAS TASK FORCE Ray Egerton ,Charles E. Fiori ,John A. Hunt, Mike S. Isaacson,Earl J. Kirkland ,Nestor J. Zaluzec Correspondence Address :R.F. EGERTON-CHAIRMAN University of Alberta Dept. of Physics Edmonton, Alberta, Canada, T6G2J1 Abstract:
A simple format for the exchange of digital spectral data is presented, and proposed as an EMSA/MAS standard. This format is readable by both humans and computers and is suitable for transmission through various electronic networks (BITNET, ARPANET), the phone system (with modems) or on physical computer storage devices (such as floppy disks). The format is not tied to any one computer, programming language or computer operating system. The adoption of a standard format would enable different laboratories to freely exchange spectral data, and would help to standarize data analysis software. If equipment manufacturers were to support a common format, the microscopy and microanalysis community would avoid duplicated effort in writing data-analysis software. This version of EMSAMASFF contains two subroutines which read and write spectral data files Version 1.0 data format. The data are stored as simple ASCII characters at a user defined number of columns per line for the length of the data file. The spectral data is preceeded by a series of header lines, which tell the user about the parameters of the spectrum. The header lines are identified by the first character in the line being the symbol (#) followed by a descriptor and if appropriate its units. An example of a data file format can be found in the EMSAMASFF.DOC file.
I use EDTA with NaOH to decalcify, it's slow and you have to keep it cold, but it is gentle. Then dehydrate and infiltrate with long spells in each change, and embed in a hard resin - I use Epon with DDSA and NMA and, to embed, 2% DMP30. Use vacuum or a rotator (or both in turn) to force the resin in, and after embedding leave it overnight at 37C, if possible under vacuum (I use an old paraffin oven) before putting it into the 60C oven. People do use microwave techniques, but I never had much luck with them. Hope this helps.
Lesley Weston.
on 03/05/2002 1:36 PM, Jo Dee Fish at jfish-at-gladstone.ucsf.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 } -----------------------------------------------------------------------. } } } Hello microscopists, } I am looking for a tried and true protocol for mouse bone. We are } interested in looking at the osteoblasts, and I am not sure how to } preserve them for examination of ultrathin sections in the TEM. } What is the best decalcification method? What type of resin for } embedding? Would a low viscosity resin, such as Spurr's, be the best? } I would appreciate any help you could give. } Thanks, } Jo Dee Fish } } ************************************************************ } Jo Dee Fish } Research Technologist II } Microscopy Core } Gladstone Institute of Cardiovascular Disease } } Telephone: (415) 695-3720 } Fax: (415) 285-5632 } E-mail: jfish-at-gladstone.ucsf.edu } } Mailing address: } Gladstone Institutes } P.O. Box 419100 } San Francisco, CA 94141-9100 } ************************************************************ }
I think that you have a need to trust your analyst to know what he/she is doing. Unfortunately, in the age of push button data collection on instruments that anyone can use, the training may or may not be up to snuff. Of course, you can rely on "certified" labs that are ISO-9000 qualified, but if you do, they may be just following a rote script. It is best to know that analyst's pedigree and their experience level.
-Scott
Scott D. Walck, Ph.D. PPG Industries, Inc. Glass Technology Center P. O. Box 11472 (letters) Guys Run Rd. (packages) Pittsburgh, PA 15238-0472
Walck-at-PPG.com
(412) 820-8651 (office) (412) 820-8515 (fax)
-----Original Message----- } From: Peter Tomic [mailto:PTomic-at-anadigics.com] Sent: Friday, May 03, 2002 11:20 PM To: Microscopy-at-sparc5.microscopy.com
Folks;
On a few occasions I have been handed reports from outside our organization with EDX spectra that were saved as image files, e.g. .bmp. .tif, .jpg etc. and pasted into a Word document or another report format. However, this "cut and paste job" is only an image and in my mind isn't data at all but simply information that can't be verified or refuted. A case in point is when I received a spectra that only displayed energies up to 3.5 KeV and the report identified Pt as Au which overlap at the lower energy region but spread out higher up. Now without the raw data I cannot do anything but take someone's word or politely interrogate the person that did the analysis. My question is whether it would be appropriate to ask someone on this listserver with the same EDX system to look at the raw data, if available, provided they have the same platform?
These matters are generally not life and death like a forensics issue but purely economic, but I'd rather be in jail than lose money.
Unfortunately sometimes the "analyst" is a few people removed in the food chain of the organization I may have to deal with and that's sometimes a customer so I must at all times be cordial and diplomatic. It turned out that the individual that sent me the "pictorial" spectra, but no raw data, was a "push button" let the machine identify everything type of analyst and was not very conversant in where error comes from in EDX analyses. He also had no real understanding of the device he was "analyzing" so I should probably be a bit more forgiving. I would have preferred that his report stated "these are the possible elements detected, Au, Pt etc."
I must take this opportunity to agree with you on ISO9000 certification and speak my mind. ISO is not an education in engineering or science, it is an education on how to be compliant with paperwork. If one documents a bad recipe for a cake, one will get a consistently bad cake but will not be on The Martha Stewart Show. I often wonder how many organizations filed for bankruptcy but had wonderful ISO documentation and passed all their audits? I really should look this up somewhere.
I hope my boss doesn't subscribe to this, naaaaah.
Peter
-----Original Message----- } From: Walck, Scott D. [mailto:walck-at-ppg.com] Sent: Saturday, May 04, 2002 4:25 PM To: 'Peter Tomic' Cc: Microscopy (E-mail)
Folks;
On a few occasions I have been handed reports from outside our organization with EDX spectra that were saved as image files, e.g. .bmp. .tif, .jpg etc. and pasted into a Word document or another report format. However, this "cut and paste job" is only an image and in my mind isn't data at all but simply information that can't be verified or refuted. A case in point is when I received a spectra that only displayed energies up to 3.5 KeV and the report identified Pt as Au which overlap at the lower energy region but spread out higher up. Now without the raw data I cannot do anything but take someone's word or politely interrogate the person that did the analysis. My question is whether it would be appropriate to ask someone on this listserver with the same EDX system to look at the raw data, if available, provided they have the same platform?
These matters are generally not life and death like a forensics issue but purely economic, but I'd rather be in jail than lose money.
At 12:01 PM -0700 on 5/3/02 you wrote: } Hi All: } I am trying to convert an image and spectra from the Oxford AN 10000 EDS } to a .tiff that is readable on a PC. I've done it in the past, but it has } been so long, I forget the exact procedure. I hope that there is } somone out there that does this more regularly that can refresh my } memory. } Thanks in advance, } Mike Coviello } UT Arlington
Procedure for converting AN10000 spectrum screendumps to TIFF format files on PC DOS disks
1) From the Analyser MAIN MENU select (4) PRINT/PLOT
2) Select (3) DUMP TO DISK Enter filename FILENAME.IM Message: File FILENAME.IM does not exist in STAFF/STUDENT.DR Do you wish to create it? Press Y The spectrum will now be saved to the working directory as FILENAME.IM
3) Return to the GO menu
4) Select (4) FILE MANAGEMENT
5) Select (16) DEMON/TIFF convert
6) Select (1) IMAGE filename. Enter FILENAME.IM
7) Select (2) TIFF filename. Enter FILENAME.TI
8) Select (3) LOOKUP table: MSDOSCV.LT
9) Select (8) IMAGE to TIFF Overwrite file if it exists: Yes Rescale pixels for grey image: Yes
10) Select (10) MSDOS convert Insert DOS formatted disk in DM0 Source disk for DOS: DM0
11) Select (1) CONVERT files Copy file to (MSDOS/DEMON): MSDOS Filename please: FILENAME.TI Any conversion type: B Transfer will now take place, lasting approximately 3 minutes. The TIFF file will be a grey-scale image. Use an image processing package to change it to color.
12) Select (3) DEMON utilities
13) Select (2) DELETE DEMON files Enter FILENAME.- Message: Delete DEMON file FILENAME.TI? Press Y Message: Delete DEMON file FILENAME.IM? Press Y Press Blue
14) Select (20) EXIT
15) Select (20) EXIT
-- Barton Smith, Ph.D. Advanced Lasers and Optics Group Engineering Science and Technology Division Oak Ridge National Laboratory
If your opinion is being sought, then you should have available all raw data. Whether it is a legalistic matter or not, a definitive opinion can not be rendered on a synopsis of available data, only on original data.
Preferably, the original sample would be made available to you for analysis. In this way, not only the interpretation, but also the providence of that interpretation would be verifiable by you.
Your query whether it is appropriate to find someone with the same equipment is moot. It is the interpretation of the results given the analytical conditions that is far more important than the data delivered. The data as delivered to you has already undergone the filters of the one who sent it to you. You need to see past that and provide your own interpretation of the truth, which can only be based on data that you know to be based on some semblance of reality. Since the data collection of EDX spectra is based on a variety of experimental conditions, the better they are known, the better they can be corrected for.
In other words, you need to know not only the raw data but also the experimental conditions it was collected under as well as the providence of the sample. To provide an opinion on anything less would be a disservice to those who ask as well as those who oppose the requesting party. Assuming the desire to be an impartial source, there is no other course than to do your own analysis..
Allen R. Sampson Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174
} } Folks; } } On a few occasions I have been handed reports from outside our organization } with EDX spectra that were saved as image files, e.g. .bmp. .tif, .jpg etc. } and pasted into a Word document or another report format. However, this } "cut and paste job" is only an image and in my mind isn't data at all but } simply information that can't be verified or refuted. A case in point is } when I received a spectra that only displayed energies up to 3.5 KeV and the } report identified Pt as Au which overlap at the lower energy region but } spread out higher up. Now without the raw data I cannot do anything but } take someone's word or politely interrogate the person that did the } analysis. My question is whether it would be appropriate to ask someone on } this listserver with the same EDX system to look at the raw data, if } available, provided they have the same platform? } } These matters are generally not life and death like a forensics issue but } purely economic, but I'd rather be in jail than lose money. } } Regards, } Peter }
Karli - by chance could your column be containmented or have a whisker? I know sometimes if your image isn't good sometimes your filament could be going, but probably not for weeks. Just a thought. Barb
I ran across an LSI-11 bus M7555 card which seems to be in good condition. No idea what it is or if it works. It has a ribbon connector (1) on the pull handles end. It is a DEC card.
Thank you. I am saving this email for reference in my next argument with upper management.
Peter
-----Original Message----- } From: Allen Sampson [mailto:ars-at-sem.com] Sent: Sunday, May 05, 2002 7:11 AM To: 'Peter Tomic'; Microscopy-at-sparc5.microscopy.com
Hi all,
I have a specific question regarding experiments in inert environment:
The experiment I did was: A small superalloy (SA) sample was taken in a quartz tube and I placed the tube horizontally in a tube furnace. I then ran Ar gas for a few minutes through it and under the assumption that all oxygen is gone, heated the tube to 1200 C, held there for 50 min before cooling the apparatus to 200C. This I thought would avoid any oxidation of the SA sample. On cooling, to my disappointment, the SA surface oxidized (shiny surface became black). In fact, the quartz tube became black from inside. Note that throughout the experiment, I had inserted a thermocouple in the quartz tube, which (the thermocouple) had a Nextel Ceramic fiber insulation. This insulation also turned black.
The specific questions in my mind are: 1) How do I make sure that all the oxygen is flushed out? Is a vacuum necessary before Ar gas is filled in the tube? 2) In my experiment, did the Thermocouple insulation emit any gas (from the black color of the quartz tube and the nextel insulation)? In that case, can i have a bare theomocouple wire in the tube at 1200C?
Thanks in advance
Rahul Panat Dept. of Theoretical and Applied Mechanics Univ of Illinois, Urbana, IL
on 5/5/02 10:11 PM, rahul padmakar panat at panat-at-students.uiuc.edu wrote:
} } I have a specific question regarding experiments in inert environment: } } The experiment I did was: A small superalloy (SA) sample was taken } in a quartz tube and I placed the tube horizontally in a tube furnace. I } then ran Ar gas for a few minutes through it and under the assumption } that all oxygen is gone, heated the tube to 1200 C, held there for 50 } min before cooling the apparatus to 200C. This I thought would avoid } any oxidation of the SA sample. } On cooling, to my disappointment, the SA surface } oxidized (shiny surface became black). In fact, the quartz tube became } black from inside. Note that throughout the experiment, I had inserted } a thermocouple in the quartz tube, which (the thermocouple) had a Nextel } Ceramic fiber insulation. This insulation also turned black. } } The specific questions in my mind are: } 1) How do I make sure that all the oxygen is flushed out? Is a } vacuum necessary before Ar gas is filled in the tube? } 2) In my experiment, did the Thermocouple insulation emit any gas (from } the black color of the quartz tube and the nextel insulation)? } In that case, can i have a bare theomocouple wire in the tube at } 1200C? } } Thanks in advance } } Rahul Panat } Dear Rahul, If you had a long, thin quartz tube, the Ar would not necessarily flush out all the O2, so, yes, I would evacuate the tube furnace, flush with Ar, repeat until all the O2 is gone. (I'm thinking that the tube was not open at both ends, and that the Ar was not directed at the end of the tube.) I'd try the experiment again without the SA, but with a clean quartz tube and new TC; if they again turn black, then it's something in the TC insulation. If not, try again with the SA, and see if anything unexpected occurs. Good luck. Yours, Bill Tivol
We normally imbed in gelatin capsules. Polymerise in a oven. Use a hacksaw (Very small) to cut and re-glue our specimens in the preferred orientation before sectioning. That way our orientation is perfect every time!
Just a useful hint.
Mr S. H. Coetzee Electron Microscope Unit University of Botswana Private Bag 0022 Gabarone Botswana
-----Original Message----- } From: Ann-Fook Yang [mailto:yanga-at-EM.AGR.CA] Sent: Friday, May 03, 2002 5:26 PM To: microscopy-at-sparc5.microscopy.com
Hi everyone,
I need to do flat embedding using LR White. A Teflon mold covered with ACLAR seems to be the answer. I am afraid that the over filled resin under ACLAR may not polimerize properly and become messy. I appreciate your experience.
We have a Jeol 100CX TEM that, I am told, has developed the following vacuum problem over the last 5-7 years. The problem, whatever its cause, means that the viewing port into the observation chamber has to be removed once a month or so to clean off the buildup of oil on the inside. I am amazed that this was considered Ok for the microscope........ So, my proposal is to replace all the rubber vacuum lines, and clean out, as best as possible, the remaining components - metal hoses, etc. We're not sure of the cause of this problem, whether it's oil from the rotary pumps or from one of the diffusion pumps. Oh, and we need to clean, or at least check, the column as well, of course......
My questions are: Can we replace the original rubber tubing with wire-reinforced clear PVC tubing (at least then we'd see any oil buildup in future)? It's a little unclear how much vacuum the PVC tubing will take and this will be important in the internals of the microscope.
How can we identify the source of the problem? I'm proposing to put foreline traps on both rotary pumps, but if a diff pump is the problem, this won't solve it. I'm also proposing to take out the diff pumps and check them, change the oil, etc. I've had a look through Will Bigelow's Vacuum Methods book (very useful!), and it's a bit like reading an index of diseases and their symptoms - you think you have a whole variety of them!! - I can see several incidents and problems that could have affected a number of the vacuum components.
Thanks for any and all advice! cheers, Rosemary
Rosemary White Microscopy Centre CSIRO Plant Industry GPO Box 1600 Canberra, ACT 2601 Australia
61- 2 6246 5475 or 61- 0402 835 973 rosemary.white-at-csiro.au
Yes, a changeover to the clear PVC hosing is appropriate - I love the stuff. The problem you are experiencing is probably more a consequence of the calibration of the vacuum system than anything else.
Anyone who has been here for awhile has probably seen postings from me on the vacuum system calibrations of EMs regarding the cross-over points of diffusion pumped systems. Too often, design engineered or field engineering solutions result in a cross-over vacuum level from roughing to diffusion pumps at too high a pressure level. When a diffusion pump is opened to a pressure level too high, it can stall which results in the breakdown of the normal laminar flow of oil vapor to a chaotic flow which results in the influx of oil vapor into the sample chamber.
Your first step should be to determine the actual chamber pressure at which the cross-over from roughing to diffusion pump occurs. At the least, you can get a qualitative determination from the action of the chamber vacuum when the diffusion pump kicks in. At that point, the vacuum level should start a rapid increase to the ultimate vacuum. If, instead, the vacuum level declines or holds steady for a few seconds, the cross-over point is too high and the diffusion pump is stalling. Cross-over should normally occur at 70 - 100 microns, most diffusion pumps will react well in this area. I generally tend to set the cross-over at 70 microns - it will take longer for the roughing time but when the diffusion pump kicks in it will rapidly pull down to the ultimate vacuum and the sample chamber will remain cleaner.
Field engineers don't normally carry independant vacuum measuring gear. Instead, they depend on known timing characteristics of known good systems. If your system doesn't match the characteristics expected, the calibration will be off. The only offset to this is the use of a leak back test, where the actual leak rate of the system can be tested. If the leak back can be verified as within the manufacturer's specs, then the calibration can be applied and expected to achieve specs.
If, however, there is no absolute measurement made of either actual vacuum levels or actual leak rates, then no assumptions can possibly be made of the vacuum levels achieved. Turbo-pumping systems actually make this determination of vacuum levels more problematic as they are seldom capable of closing a valve on the sample chamber to allow the determination of its leak rate, making the use of accurate vacuum level measuring equipment neccessary to determining the the calibration of system levels.
Allen R. Sampson Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174
On Sunday, May 05, 2002 11:50 PM, Rosemary White [SMTP:rosemary.white-at-csiro.au] wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Dear all, } } We have a Jeol 100CX TEM that, I am told, has developed the following } vacuum problem over the last 5-7 years. The problem, whatever its cause, } means that the viewing port into the observation chamber has to be removed } once a month or so to clean off the buildup of oil on the inside. I am } amazed that this was considered Ok for the microscope........ So, my } proposal is to replace all the rubber vacuum lines, and clean out, as best } as possible, the remaining components - metal hoses, etc. We're not sure } of the cause of this problem, whether it's oil from the rotary pumps or } from one of the diffusion pumps. Oh, and we need to clean, or at least } check, the column as well, of course...... } } My questions are: } Can we replace the original rubber tubing with wire-reinforced clear PVC } tubing (at least then we'd see any oil buildup in future)? It's a little } unclear how much vacuum the PVC tubing will take and this will be important } in the internals of the microscope. } } How can we identify the source of the problem? I'm proposing to put } foreline traps on both rotary pumps, but if a diff pump is the problem, } this won't solve it. I'm also proposing to take out the diff pumps and } check them, change the oil, etc. I've had a look through Will Bigelow's } Vacuum Methods book (very useful!), and it's a bit like reading an index of } diseases and their symptoms - you think you have a whole variety of them!! } - I can see several incidents and problems that could have affected a } number of the vacuum components. } } } Thanks for any and all advice! } cheers, } Rosemary } } Rosemary White } Microscopy Centre } CSIRO Plant Industry } GPO Box 1600 } Canberra, ACT 2601 } Australia } } 61- 2 6246 5475 or } 61- 0402 835 973 } rosemary.white-at-csiro.au } } } } }
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I received the below notice from our friendly IT people. I believe it was incoming from the listserver and I though you may want to be cautious about the "sender."
Regards, Peter
-----Original Message----- } From: MB10190 [mailto:MB10190-at-aol.com] Sent: Sunday, May 05, 2002 1:40 PM To: PTomic-at-anadigics.com
I would add; verify purity of your argon or use an argon purifier.
At 8:40 PM -0400 5/5/02, Bill & Sue Tivol wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
-- David R. Hull NASA Glenn Research Center at Lewis Field Advanced Metallics Branch Mail Stop 49-1 21000 Brookpark Road Cleveland, OH 44135
My approaches in using LRWhite differ by the nature of the sample being embedded: Hard samples, such as silica and zeolites, are embedded in LRWhite (hard grade) without accelerator. The sample is first vacuum degassed, immersed in LRWhite in the mold and placed under vacuum again to facilitate complete infiltration of the resin into the sample. The embedded sample is then cured overnight at 75-90C. This gives a hard, brittle block that is ideal for sectioning hard samples. I try to avoid embeddment of polymers in LRWhite. Some polymers may be partially to very soluble in the acrylic monomer and thus susceptible to swelling by the resin. Furthermore, since the heat of curing is not known to me, I choose not to take chances on the annealing samples during exothermic curing. Rather, I generally choose to use one of the generic Epon 812 replacements for these materials. Carefully controlled curing conditions allow embedment and microtomy without concerns of annealing. This said, if I must embed polymers in LRWhite, I choose the correct hardness of resin (soft, medium or hard) for the material being embedded. The embedding mold is degassed for a bit under a nitrogen flow and the mold surfaces are then wiped with the accelerant on a cotton swab. This helps the resin in contact with the mold surface to more fully cure. The samples are embedded in the resin/accelerator and immediately placed under nitrogen flow until curing is complete.
Good luck,
Gary M. Brown
"Ann-Fook Yang" {yanga-at-EM.AGR.C To: {microscopy-at-sparc5.microscopy.com} A} cc: Subject: Flat embedding of LR White
05/03/02 10:26 AM
------------------------------------------------------------------------ The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Hi everyone,
I need to do flat embedding using LR White. A Teflon mold covered with ACLAR seems to be the answer. I am afraid that the over filled resin under ACLAR may not polimerize properly and become messy. I appreciate your experience.
I'm glad someone else got around to this before I did! As you can see, it's rather involved. I will add two additional points:
1) One of my AN10000's doesn't have DEMON/TIFF convert as an option (older software). I must use the "newer" version of the QX200 Utilities software. 2) At step 9 below: both answers must be an uppercase 'Y'. Again, possibly peculiar to my system/version. Good luck!
Matt
Matthew J. Lynn Center for Advanced Microscopy University of Miami (305)284-4736 mlynn-at-miami.edu
On Saturday, May 04, 2002 7:58 PM, Barton Smith [SMTP:smithdb-at-ornl.gov] 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.ht } ml } ---------------------------------------------------------- } -------------. } } } At 12:01 PM -0700 on 5/3/02 you wrote: } } Hi All: } } I am trying to convert an image and spectra from the } } Oxford AN 10000 EDS } } to a .tiff that is readable on a PC. I've done it in the } } past, but it has } } been so long, I forget the exact procedure. I hope that } } there is } } somone out there that does this more regularly that can } } refresh my } } memory. } } Thanks in advance, } } Mike Coviello } } UT Arlington } } } Procedure for converting AN10000 spectrum screendumps to } TIFF format } files on PC DOS disks } } 1) From the Analyser MAIN MENU select (4) PRINT/PLOT } } 2) Select (3) DUMP TO DISK } Enter filename FILENAME.IM } Message: File FILENAME.IM does not exist in } STAFF/STUDENT.DR } Do you wish to create it? Press Y } The spectrum will now be saved to the working directory } as FILENAME.IM } } 3) Return to the GO menu } } 4) Select (4) FILE MANAGEMENT } } 5) Select (16) DEMON/TIFF convert } } 6) Select (1) IMAGE filename. Enter FILENAME.IM } } 7) Select (2) TIFF filename. Enter FILENAME.TI } } 8) Select (3) LOOKUP table: MSDOSCV.LT } } 9) Select (8) IMAGE to TIFF } Overwrite file if it exists: Yes } Rescale pixels for grey image: Yes } } 10) Select (10) MSDOS convert } Insert DOS formatted disk in DM0 } Source disk for DOS: DM0 } } 11) Select (1) CONVERT files } Copy file to (MSDOS/DEMON): MSDOS } Filename please: FILENAME.TI } Any conversion type: B } Transfer will now take place, lasting approximately 3 } minutes. The TIFF file will be a } grey-scale image. Use an image processing } package to } change it to color. } } 12) Select (3) DEMON utilities } } 13) Select (2) DELETE DEMON files } Enter FILENAME.- } Message: Delete DEMON file FILENAME.TI? Press Y } Message: Delete DEMON file FILENAME.IM? Press Y } Press Blue } } 14) Select (20) EXIT } } 15) Select (20) EXIT } } } } -- } Barton Smith, Ph.D. } Advanced Lasers and Optics Group } Engineering Science and Technology Division } Oak Ridge National Laboratory
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Dear Rahul Panat
If it is possible link the tube to a vacuum system it will help. Flushing with Ar a few times will improve it dramatically. It is worth to allow a very slow flow of Ar during heating and cooling over your sample. This is done by closing both ends of your quarts tube with a inlet and outlet pipe. The outlet pipe is run into a holder with water. Increase the Ar flow until a very small bubble rate is achieved. This will ensure a inert atmosphere with a positive Ar pressure.
Yours Sincerely Stephan H. Coetzee Electron Microscope Unit University of Botswana Private Bag 0022 Gabarone Botswana
I have a specific question regarding experiments in inert environment:
The experiment I did was: A small superalloy (SA) sample was taken in a quartz tube and I placed the tube horizontally in a tube furnace. I then ran Ar gas for a few minutes through it and under the assumption that all oxygen is gone, heated the tube to 1200 C, held there for 50 min before cooling the apparatus to 200C. This I thought would avoid any oxidation of the SA sample. On cooling, to my disappointment, the SA surface oxidized (shiny surface became black). In fact, the quartz tube became black from inside. Note that throughout the experiment, I had inserted a thermocouple in the quartz tube, which (the thermocouple) had a Nextel Ceramic fiber insulation. This insulation also turned black.
The specific questions in my mind are: 1) How do I make sure that all the oxygen is flushed out? Is a vacuum necessary before Ar gas is filled in the tube? 2) In my experiment, did the Thermocouple insulation emit any gas (from the black color of the quartz tube and the nextel insulation)? In that case, can i have a bare theomocouple wire in the tube at 1200C?
Thanks in advance
Rahul Panat Dept. of Theoretical and Applied Mechanics Univ of Illinois, Urbana, IL
From root Mon May 6 15:37:48 2002 Return-Path: {Microscopy-request-at-sparc5.microscopy.com} Received: (from daemon-at-localhost) by sparc5.microscopy.com (8.9.3+Sun/8.9.3) id PAA20294 for dist-Microscopy; Mon, 6 May 2002 15:20:42 -0500 (CDT) Received: from njz_spm_filter (sparc5 [206.69.208.10]) by sparc5.microscopy.com (8.9.3+Sun/8.9.3) with SMTP id PAA20288 for "MicroscopyFilteredEmail1-at-msa.microscopy.com"; Mon, 6 May 2002 15:20:12 -0500 (CDT) Received: from jhuml2.jhmi.edu ([162.129.234.21]) by sparc5.microscopy.com (8.9.3+Sun/8.9.3) with ESMTP id PAA20279 for {Microscopy-at-sparc5.microscopy.com} ; Mon, 6 May 2002 15:19:54 -0500 (CDT) Received: from jhuml2.jhmi.edu (jhuml2.jhmi.edu [162.129.234.21]) by jhuml2.jhmi.edu (PMDF V6.1 #47568) with SMTP id {0GVP00BK1HL9VL-at-jhuml2.jhmi.edu} for Microscopy-at-sparc5.microscopy.com; Mon, 06 May 2002 16:15:19 -0400 (EDT) Received: from jhuml2.jhmi.edu ([162.129.234.21]) by jhuml2.jhmi.edu (NAVGW 2.5.1.18) with SMTP id M2002050616151912152 for {Microscopy-at-sparc5.microscopy.com} ; Mon, 06 May 2002 16:15:19 -0400 Received: from jhem2.jhmi.edu (jhem2.jhmi.edu [162.129.8.23]) by jhuml2.jhmi.edu (PMDF V6.1 #47568) with ESMTP id {0GVP00BL2HLJVL-at-jhuml2.jhmi.edu} for Microscopy-at-sparc5.microscopy.com; Mon, 06 May 2002 16:15:19 -0400 (EDT) Received: from jhem.jhmi.edu (MicfacG3.dhcp.bs.som.jhmi.edu [162.129.34.158]) by jhmimail.jhmi.edu (iPlanet Messaging Server 5.2 (built Feb 21 2002)) with ESMTPA id {0GVP00GTVHR8DO-at-jhmimail.jhmi.edu} for Microscopy-at-sparc5.microscopy.com; Mon, 06 May 2002 16:18:44 -0400 (EDT)
Pauline, Try decreasing the brighter labels concentration. Also run single label counterparts as bleed through controls (same concentrations as the double label, but use only the fitc and PI separately). If you get bleed with the single label samples (capture with both channels), you can then do a backround subtract to get the real signal. Good luck
Mike D.
pcy wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } We have stained annelid embryos with FITC-conjugated anti-tubulin antibody } and propidium iodide. We are using a Biorad-MRC-600 and seem to be getting } almost identical signals(of nuclei and a few mitochondria) on both the 488 } and 568 wavelengths, even though when viewed with epifluorescence, the } tubulin stain seems to distinctly define cell borders. I understood that } the propidium iodide emission would not be overlapping with that of } FITC--is this incorrect? I have other double-labelled samples which are } stained with different stains, but their signals are within the } appropriate emission spectra for both confocal and epifluorescence, so the } detection filters on the confocal do not seem to be the problem. } } Any feedback is appreciated! } } Pauline Yu } pcy-at-usc.edu } Manahan Lab } http://www.usc.edu/manahanlab
} Date: Mon, 06 May 2002 14:39:09 -0700 } To: "ars-at-sem.com" {ars-at-sem.com} } From: Sergey Ryazantsev {sryazant-at-ucla.edu} } Subject: RE: cleaning vacuum system } } The only things you have to keep in mind: PVC tubes are less flexible and } may 'transfer' vibration from rotary pump to the microscope's column. For } this reason, I love to use PVC on vacuum evaporators nor the microscopes. } } As for oil in the column - to me it looks like DP problem and water } waffler, which is situate over DP. The reason I think so, that usually we } do not pump columns down by RP very often. It happening on my microscope } a few times over 15 years, I believe. So, it mean, that RP do not touch } column frequently (except terrible downstream if it happening). I do } believe that 100C/CX DPs have water wafflers, check does water go } through. Another things: if DP oil is old (or overheated over some period } of time) it may be deteriorated and boiling point may decreased (shorter } molecules), so some low-weight components may not condensate effectively } and will migrate into the column. I would suggest to check DP oil and } replace it on Santovak-5 like type (and forget for 5+ years). If you } decided to replace DP oil, I would suggest, you install oil traps on RPs } and new tubings as well to protect fresh oil (you never know...). Good } luck! Sergey } } At 05:04 AM 5/6/02 -0700, you wrote: } } ------------------------------------------------------------------------ } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
After all the cleaning, I would check the water lines & the water temperature.
I have had problems similar to the one you describe. It turned out that after moving the EM the input & output lines were reversed causing oil backstreaming. In the second case, the water temperature had increased overnight as it was connected to the tap water.
Another thought would be to check the pre-pump pressure to ensure that it is switching over at the correct pressure.
Regards,
Earl
----- Original Message ----- } From: "Rosemary White" {rosemary.white-at-csiro.au} To: {Microscopy-at-sparc5.microscopy.com} Sent: Sunday, May 05, 2002 11:49 PM
Dear Rosemary
Once, in the darkness of time (1975-...), I used one of the first JEOL 100C microscopes. That machine also developed with time severe contamination problems that, I believe, may be similar to the ones you mention. As far as we could find out, and as far as I can recall (forgive some possible innacuracies) the trouble came from the particular design of the vacum system, in which two diffusion pumps are linked together, the exit of the upper pump being connected to the observation chamber. In these early microscopes, that design seemed to lead to oil reflux from the exit of the upper pump into the column, at least during some stages of the vacum sequence. One cure for the problem was to close permanently the valve connecting the observation chamber with the vacuum system. That was the only measure that worked! Enough vacuum could still be achieved by the upper connection alone. As far as I was told newer microscopes (yours should be one of these) were built with an improved automated vacuum sequence and traps that avoided that problem. My guess is that either your oil traps are not operational (obstructed water circulation?), either the vacuum sequence is incorrect (check the pirani gauge settings that control the sequence against true vacum values if you are able to measure them!). Some vacuum valve (the lower connection to the column should be the primary suspect) may be stuck, or electronics is producing a wrong sequence etc... Anyhow if you have this problem, continuos cleaning does not seem to be an answer. It was not for me.
Best wishes and good luck Prof. Doctor A.P. Alves de Matos Anatomic Pathology Department Curry Cabral Hospital Lisbon
-----Mensagem original----- De: Rosemary White [mailto:rosemary.white-at-csiro.au] Enviada: Segunda-feira, 6 de Maio de 2002 7:50 Para: Microscopy-at-sparc5.microscopy.com Assunto: cleaning vacuum system
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Dear all,
We have a Jeol 100CX TEM that, I am told, has developed the following vacuum problem over the last 5-7 years. The problem, whatever its cause, means that the viewing port into the observation chamber has to be removed once a month or so to clean off the buildup of oil on the inside. I am amazed that this was considered Ok for the microscope........ So, my proposal is to replace all the rubber vacuum lines, and clean out, as best as possible, the remaining components - metal hoses, etc. We're not sure of the cause of this problem, whether it's oil from the rotary pumps or from one of the diffusion pumps. Oh, and we need to clean, or at least check, the column as well, of course......
My questions are: Can we replace the original rubber tubing with wire-reinforced clear PVC tubing (at least then we'd see any oil buildup in future)? It's a little unclear how much vacuum the PVC tubing will take and this will be important in the internals of the microscope.
How can we identify the source of the problem? I'm proposing to put foreline traps on both rotary pumps, but if a diff pump is the problem, this won't solve it. I'm also proposing to take out the diff pumps and check them, change the oil, etc. I've had a look through Will Bigelow's Vacuum Methods book (very useful!), and it's a bit like reading an index of diseases and their symptoms - you think you have a whole variety of them!! - I can see several incidents and problems that could have affected a number of the vacuum components.
Thanks for any and all advice! cheers, Rosemary
Rosemary White Microscopy Centre CSIRO Plant Industry GPO Box 1600 Canberra, ACT 2601 Australia
61- 2 6246 5475 or 61- 0402 835 973 rosemary.white-at-csiro.au
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MICROSCOPY TODAY, May/June 2002 __________________________ Index of Articles __________________________
Food Under The Microscope Stephen Carmichael, Mayo Clinic
Some Thoughts On Vibrations In EM Laboratories Anthony J. Garratt-Reed, MIT
The Emergence of Aberration Correctors for Electron Lenses John Silcox, Cornell University
Fast OIM D. J. Dingley*, S. Wright and M. Nowell TSL (a subsidiary of EDAX)
Fitting a Student Microscope with a Consumer Digital Camera Theodore M. Clarke, Metallurgical F. A. Consultant
Microscopy in the Real World: A Manufacturer's Perspective Michael M. Kersker, JEOL USA, Inc.
All That Glitters is not Gold: Approaches to Labeling for TEM R.M. Albrecht and D.A. Meyer, University of Wisconsin
Low Voltage Scanning Electron Microscopy and Jack Ramsey's principle Oliver C. Wells, IBM Research Division
More on the Calibration of TEMs J. P. McCaffrey, N.R.C. and R. Beanland, Bookham Technology PLC
Lateral Resolution in Scanning Force Microscopy Brian A. Todd and Steven J. Eppell Case Western Reserve University
Utilizing Original TEM Negatives and Micrographs For Teaching in the Digital Domain José A. Mascorro, Tulane University
Plunge-Freezing into Slush Nitrogen Philip Oshel, University of Wisconsin
Downloadable Photoshop Convolution Plug-In John Russ, North Carolina State University
A Home-made Antifade Medium for Fluorescent Dyes Tim Plummer, Mayo Clinic
A few people suggested checking the water cooling system - we had to replace the chiller last year, and we're replacing the water lines now at the same time as we replace the vacuum lines in this overhaul - there are a couple of very slow water leaks and some of the old rubber water lines are very stiff. Our water tends to be on the cool side rather than too hot - never more than 20C, though we did have a period of about a week or two after the new chiller went in when the water got up to 24-25C. And all the EMs were on tap water for about 6 months while we waited for the new chiller....... But the oil problem started long before this.
The amazing thing about this TEM is that the image quality is pretty good. However, some oil (or something) has definitely got into the column because during an EM maintenance training session last year, we took the top off the column and cleaned the upper chamber and gun - the inside of the chamber was brown! However, since this was its first clean in at least 12 years, perhaps this isn't surprising. The TEM itself is 25 years old (so the diff pump oil is also 25 years old) and has been in this building for 12 years. It may be that the move to this building caused a minor leak somewhere in the system.
The guys have just started taking the diff pumps out, and we can see oil leaking out of the solenoids on the vacuum system at the back of the column..... We're all going to have fun, I can see!!!
Once it's clean and put back together, we'll follow Allen Sampson's suggestion re. checking the cross-over vacuum setting.
cheers, Rosemary
Rosemary White Microscopy Centre CSIRO Plant Industry GPO Box 1600 Canberra, ACT 2601 Australia
61- 2 6246 5475 or 61- 0402 835 973 rosemary.white-at-csiro.au
I met a problem about the AFM images. As you know, although there is no real meaning of 3-D image in AFM, it is a good format to show the AFM result. But the thing is: How to make two images have the same Z value?
My AFM system is the ThermoMicroscope. The software I use is Proscan. Could somebody help me to find out how to get the same Z value for different images out of my system? Or could you introduce another reasonable software for me?
Looking forward for your help!
Yours, Xianglin Li
Center for Advanced Material Department of Chemical Engineering University of Massachusetts, Lowell Xianglin_Li-at-student.uml.edu Tel: 978-934-3411
As far as the PVC tubing, I have rarely seen cases where the proper installation of roughing pump tubing of any kind induces a significant vibration problem. Far more common are the building vibrations induced through the structural members of the EM. However, I did qualify that as a proper installation of the tubing. Case in point - one manufacturer's service rep who replaced the tubing from the optics table to the vibration isolator (the lead or concrete filled block usually used to dampen vibrations). He added around 8 feet of extra tubing that he left coiled on the floor claiming that it was known that that length of tubing was required to reduce vibrations. Needless to say, when the excess was removed the customer was greatly relieved that his FESEM actually could image above 20KX.
Old DP oil can be a problem and the original poster has admitted to an inordinate amount of time between changes. I assumed changes around 5 years and am culpable once again for the assumption that the service organizations are doing their business properly and an apparently aware operator would be apprised of the timing of good maintenance. Mea culpa.
Santovac 5 another one of my favorites. Anyone who knows me knows that I am reluctant to endorse any particular product or service, but you've hit two of my favorites in one posting and I can't help it.
You also bring up another pet peeve of mine - improperly placed foreline traps. A foreline trap is a device that is inserted between a mechanical pump and the instrument that is designed to condense oil vapors backstreaming from the mechanical pump. Ideally, they should be placed at least a few inches from the inlet of the pump, to provide thermal isolation from the pump. A trap at room temperature will do a better job than one at an elevated temperature caused by close contact with a constantly operated pump.
The trap should be placed vertically so that the condensed oils can be drawn back into the pump by gravity. Nothing worse than being called in to fix an instrument that won't pump down only to find the foreline trap laying horizontal on the floor and it and the vacuum hose flooded with collected oil.
Allen R. Sampson Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174
On Monday, May 06, 2002 2:42 PM, Sergey Ryazantsev [SMTP:sryazant-at-ucla.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 } -----------------------------------------------------------------------. } } } } } Date: Mon, 06 May 2002 14:39:09 -0700 } } To: "ars-at-sem.com" {ars-at-sem.com} } } From: Sergey Ryazantsev {sryazant-at-ucla.edu} } } Subject: RE: cleaning vacuum system } } } } The only things you have to keep in mind: PVC tubes are less flexible and } } may 'transfer' vibration from rotary pump to the microscope's column. For } } this reason, I love to use PVC on vacuum evaporators nor the microscopes. } } } } As for oil in the column - to me it looks like DP problem and water } } waffler, which is situate over DP. The reason I think so, that usually we } } do not pump columns down by RP very often. It happening on my microscope } } a few times over 15 years, I believe. So, it mean, that RP do not touch } } column frequently (except terrible downstream if it happening). I do } } believe that 100C/CX DPs have water wafflers, check does water go } } through. Another things: if DP oil is old (or overheated over some period } } of time) it may be deteriorated and boiling point may decreased (shorter } } molecules), so some low-weight components may not condensate effectively } } and will migrate into the column. I would suggest to check DP oil and } } replace it on Santovak-5 like type (and forget for 5+ years). If you } } decided to replace DP oil, I would suggest, you install oil traps on RPs } } and new tubings as well to protect fresh oil (you never know...). Good } } luck! Sergey } } } } At 05:04 AM 5/6/02 -0700, 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 } } } -----------------------------------------------------------------------. } } } } } } } } } Yes, a changeover to the clear PVC hosing is appropriate - I love the } } } stuff. The problem you are experiencing is probably more a consequence of } } } the calibration of the vacuum system than anything else. } } } } } } Anyone who has been here for awhile has probably seen postings from me on } } } the vacuum system calibrations of EMs regarding the cross-over points of } } } diffusion pumped systems. Too often, design engineered or field } } } engineering solutions result in a cross-over vacuum level from roughing to } } } diffusion pumps at too high a pressure level. When a diffusion pump is } } } opened to a pressure level too high, it can stall which results in the } } } breakdown of the normal laminar flow of oil vapor to a chaotic flow which } } } results in the influx of oil vapor into the sample chamber. } } } } } } Your first step should be to determine the actual chamber pressure at which } } } the cross-over from roughing to diffusion pump occurs. At the least, you } } } can get a qualitative determination from the action of the chamber vacuum } } } when the diffusion pump kicks in. At that point, the vacuum level should } } } start a rapid increase to the ultimate vacuum. If, instead, the vacuum } } } level declines or holds steady for a few seconds, the cross-over point is } } } too high and the diffusion pump is stalling. Cross-over should normally } } } occur at 70 - 100 microns, most diffusion pumps will react well in this } } } area. I generally tend to set the cross-over at 70 microns - it will take } } } longer for the roughing time but when the diffusion pump kicks in it will } } } rapidly pull down to the ultimate vacuum and the sample chamber will remain } } } cleaner. } } } } } } Field engineers don't normally carry independant vacuum measuring gear. } } } Instead, they depend on known timing characteristics of known good } } } systems. If your system doesn't match the characteristics expected, the } } } calibration will be off. The only offset to this is the use of a leak back } } } test, where the actual leak rate of the system can be tested. If the leak } } } back can be verified as within the manufacturer's specs, then the } } } calibration can be applied and expected to achieve specs. } } } } } } If, however, there is no absolute measurement made of either actual vacuum } } } levels or actual leak rates, then no assumptions can possibly be made of } } } the vacuum levels achieved. Turbo-pumping systems actually make this } } } determination of vacuum levels more problematic as they are seldom capable } } } of closing a valve on the sample chamber to allow the determination of its } } } leak rate, making the use of accurate vacuum level measuring equipment } } } neccessary to determining the the calibration of system levels. } } } } } } } } } } } } Allen R. Sampson } } } Advanced Research Systems } } } 317 North 4th. Street } } } St. Charles, Illinois 60174 } } } } } } phone (630) 513-7093 fax (630) 513-7092 http://www.sem.com } } } } } } } } } On Sunday, May 05, 2002 11:50 PM, Rosemary White } } } [SMTP:rosemary.white-at-csiro.au] wrote: } } } } ------------------------------------------------------------------------ } } } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } } } } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } } } } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } } } } -----------------------------------------------------------------------. } } } } } } } } } } } } Dear all, } } } } } } } } We have a Jeol 100CX TEM that, I am told, has developed the following } } } } vacuum problem over the last 5-7 years. The problem, whatever its cause, } } } } means that the viewing port into the observation chamber has to be } } } removed } } } } once a month or so to clean off the buildup of oil on the inside. I am } } } } amazed that this was considered Ok for the microscope........ So, my } } } } proposal is to replace all the rubber vacuum lines, and clean out, as } } } best } } } } as possible, the remaining components - metal hoses, etc. We're not sure } } } } of the cause of this problem, whether it's oil from the rotary pumps or } } } } from one of the diffusion pumps. Oh, and we need to clean, or at least } } } } check, the column as well, of course...... } } } } } } } } My questions are: } } } } Can we replace the original rubber tubing with wire-reinforced clear PVC } } } } tubing (at least then we'd see any oil buildup in future)? It's a little } } } } unclear how much vacuum the PVC tubing will take and this will be } } } important } } } } in the internals of the microscope. } } } } } } } } How can we identify the source of the problem? I'm proposing to put } } } } foreline traps on both rotary pumps, but if a diff pump is the problem, } } } } this won't solve it. I'm also proposing to take out the diff pumps and } } } } check them, change the oil, etc. I've had a look through Will Bigelow's } } } } Vacuum Methods book (very useful!), and it's a bit like reading an index } } } of } } } } diseases and their symptoms - you think you have a whole variety of } } } them!! } } } } - I can see several incidents and problems that could have affected a } } } } number of the vacuum components. } } } } } } } } } } } } Thanks for any and all advice! } } } } cheers, } } } } Rosemary } } } } } } } } Rosemary White } } } } Microscopy Centre } } } } CSIRO Plant Industry } } } } GPO Box 1600 } } } } Canberra, ACT 2601 } } } } Australia } } } } } } } } 61- 2 6246 5475 or } } } } 61- 0402 835 973 } } } } rosemary.white-at-csiro.au } } } } } } } } } } } } } } } } } } } } } } } }
Has this instrument had any service at all in all those years? These instruments can be remarkable tolerant, especially if the proper supplies are used such as a DP oil that will form a non-conductive film. However, you have two choices - either make column cleanliness a regular affair where small amounts of contamination are removed at regular intervals, or make column cleanliness a rare but substantial affair where it is left alone until a problem develops and a major cleaning is required.
I have some sympathy for the task you now have, but take solace in the fact that you brought it upon yourself. What you have is one of the most sensitive and sophisticated scientific instruments ever made. Treat it in the future as the fine instrument it is and you will have many more years of happy service from it.
Allen R. Sampson Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174
On Monday, May 06, 2002 4:29 PM, Rosemary White [SMTP:rosemary.white-at-csiro.au] wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Thanks for all of your replies! } } A few people suggested checking the water cooling system - we had to } replace the chiller last year, and we're replacing the water lines now at } the same time as we replace the vacuum lines in this overhaul - there are a } couple of very slow water leaks and some of the old rubber water lines are } very stiff. Our water tends to be on the cool side rather than too hot - } never more than 20C, though we did have a period of about a week or two } after the new chiller went in when the water got up to 24-25C. And all the } EMs were on tap water for about 6 months while we waited for the new } chiller....... But the oil problem started long before this. } } The amazing thing about this TEM is that the image quality is pretty good. } However, some oil (or something) has definitely got into the column because } during an EM maintenance training session last year, we took the top off } the column and cleaned the upper chamber and gun - the inside of the } chamber was brown! However, since this was its first clean in at least 12 } years, perhaps this isn't surprising. The TEM itself is 25 years old (so } the diff pump oil is also 25 years old) and has been in this building for } 12 years. It may be that the move to this building caused a minor leak } somewhere in the system. } } The guys have just started taking the diff pumps out, and we can see oil } leaking out of the solenoids on the vacuum system at the back of the } column..... We're all going to have fun, I can see!!! } } Once it's clean and put back together, we'll follow Allen Sampson's } suggestion re. checking the cross-over vacuum setting. } } cheers, } Rosemary } } Rosemary White } Microscopy Centre } CSIRO Plant Industry } GPO Box 1600 } Canberra, ACT 2601 } Australia } } 61- 2 6246 5475 or } 61- 0402 835 973 } rosemary.white-at-csiro.au } } } } }
Yes, well this is the state the instrument was in when I arrived here 2 years ago, but was told "it's OK, it works fine, don't worry about the oil on the viewing window". As the new kid on the block and with no experience in EM maintenance, I found it hard to argue for this full overhaul. And yes, you could get OK images from it, but I still worried about the oil, so finally we are doing something about it.
The diff pumps are out now, and if any of you have looked at Fig. 5.15 in Wilbur Bigelow's Vacuum Methods book you'll have an idea what their innards looked like. The top pump had a little oil left in it, with big chunks of black goop in - and it looks like some of this junk and oil has gone further up the vacuum system. The hot parts had brown to black carbonised oil burnt firmly onto the surface. The innards of the bottom diff pump were coated in what looked like blackstrap molasses - what's left of the original oil, I guess. There was less carbonisation than in the top pump.
So, we're in for a long session, by the looks.......
Thanks again to everyone for suggestions and comments.
cheers, Rosemary
} Rosemary, you've got a lot of 'xplaining to do. } } Has this instrument had any service at all in all those years? These } instruments can be remarkable tolerant, especially if the proper supplies } are used such as a DP oil that will form a non-conductive film. However, } you have two choices - either make column cleanliness a regular affair } where small amounts of contamination are removed at regular intervals, or } make column cleanliness a rare but substantial affair where it is left } alone until a problem develops and a major cleaning is required. } } I have some sympathy for the task you now have, but take solace in the fact } that you brought it upon yourself. What you have is one of the most } sensitive and sophisticated scientific instruments ever made. Treat it in } the future as the fine instrument it is and you will have many more years } of happy service from it. } } Allen R. Sampson } Advanced Research Systems } 317 North 4th. Street } St. Charles, Illinois 60174 } } phone (630) 513-7093 fax (630) 513-7092 http://www.sem.com
Rosemary White Microscopy Centre CSIRO Plant Industry GPO Box 1600 Canberra, ACT 2601 Australia
61- 2 6246 5475 or 61- 0402 835 973 rosemary.white-at-csiro.au
Funny stuff, DP oil. Over time and use, it seems to both crack, break down into lower molecular weight products, and polymerize into larger molecular weight fractions. The polymerization generally occurs on the metallic surfaces of the pump and can only be removed by vigorous abrasive techniques (metal polish and a lot of elbow grease or sandblasting with glass beads - I haven't tried starch or CO2, but they may work). The gooey mess can normally be removed with a good detergent (Dawn dishwashing soap) or tri-chlor (not generally available anymore in the US). Mechanical buffing wheels can be helpful but be aware that some pump parts may be made of aluminum and will suffer material thinning if such means are used.
Sorry you inherited this mess. But it is a good guide to future maintenance requirements.
Allen R. Sampson Advanced Research Systems 317 North 4th. Street St. Charles, Illinois 60174
On Monday, May 06, 2002 11:43 PM, Rosemary White [SMTP:rosemary.white-at-csiro.au] wrote: } Dear Allen, } } Yes, well this is the state the instrument was in when I arrived here 2 } years ago, but was told "it's OK, it works fine, don't worry about the oil } on the viewing window". As the new kid on the block and with no } experience in EM maintenance, I found it hard to argue for this full } overhaul. And yes, you could get OK images from it, but I still worried } about the oil, so finally we are doing something about it. } } The diff pumps are out now, and if any of you have looked at Fig. 5.15 in } Wilbur Bigelow's Vacuum Methods book you'll have an idea what their innards } looked like. The top pump had a little oil left in it, with big chunks of } black goop in - and it looks like some of this junk and oil has gone } further up the vacuum system. The hot parts had brown to black carbonised } oil burnt firmly onto the surface. The innards of the bottom diff pump } were coated in what looked like blackstrap molasses - what's left of the } original oil, I guess. There was less carbonisation than in the top pump. } } So, we're in for a long session, by the looks....... } } Thanks again to everyone for suggestions and comments. } } cheers, } Rosemary } } } Rosemary, you've got a lot of 'xplaining to do. } } } } Has this instrument had any service at all in all those years? These } } instruments can be remarkable tolerant, especially if the proper supplies } } are used such as a DP oil that will form a non-conductive film. However, } } you have two choices - either make column cleanliness a regular affair } } where small amounts of contamination are removed at regular intervals, or } } make column cleanliness a rare but substantial affair where it is left } } alone until a problem develops and a major cleaning is required. } } } } I have some sympathy for the task you now have, but take solace in the fact } } that you brought it upon yourself. What you have is one of the most } } sensitive and sophisticated scientific instruments ever made. Treat it in } } the future as the fine instrument it is and you will have many more years } } of happy service from it. } } } } Allen R. Sampson } } Advanced Research Systems } } 317 North 4th. Street } } St. Charles, Illinois 60174 } } } } phone (630) 513-7093 fax (630) 513-7092 http://www.sem.com } } } Rosemary White } Microscopy Centre } CSIRO Plant Industry } GPO Box 1600 } Canberra, ACT 2601 } Australia } } 61- 2 6246 5475 or } 61- 0402 835 973 } rosemary.white-at-csiro.au } } } }
Hello, Clontech is offering a new red fluorescent Protein hcRed. Has someone made any experience using this protein. Of special interest is the question of oligomerizatin or aggregation in living cells since the older red fluorescent proteins have this tendency.
I am, and I would imagine others, are a bit confused as to what you are using the AFM for? It sounds as if you are doing a thermal map over a surface and not z-height measurements. If you are doing thermal measurements are you attempting to combine them with z-height on a surface as overlapping images?
Please elaborate and I'm sure someone can help.
Regards, Peter Tomic Anadigics, Inc.
-----Original Message----- } From: Xianglin Li [mailto:Xianglin_Li-at-student.uml.edu] Sent: Tuesday, May 07, 2002 12:00 AM To: Microscopy-at-sparc5.microscopy.com
Dear friends,
I met a problem about the AFM images. As you know, although there is no real meaning of 3-D image in AFM, it is a good format to show the AFM result. But the thing is: How to make two images have the same Z value?
My AFM system is the ThermoMicroscope. The software I use is Proscan. Could somebody help me to find out how to get the same Z value for different images out of my system? Or could you introduce another reasonable software for me?
Looking forward for your help!
Yours, Xianglin Li
Center for Advanced Material Department of Chemical Engineering University of Massachusetts, Lowell Xianglin_Li-at-student.uml.edu Tel: 978-934-3411
Mike, I had a slight memory lapse regarding Audi so I spent 5 minutes to refresh my memory. Here is a quote from The Center for Auto Safety: "With nearly 1800 reported unintended acceleration incidents in the 1980s, Audi became synonymous with the term "sudden acceleration." Despite several deaths, dozens of injuries, five related recalls and a Swedish defense agency study showing cruise control malfunctions could cause sudden acceleration, Audi claimed that "pedal misapplication" caused the incidents. Audi lost 80% of its market share because it chose to blame its customers for the problem." http://www.autosafety.org/autodefects/AUDI.htm
If memory serves me correctly one of the accidents actually occurred in a New Jersey emissions inspection station! Ouch that's likely to put a dent in your corporate image. Seems to me the free market did its job. As Sergey Ryazantsev mentioned in his reply, it is unlikely that a single negative posting will damage a credible companies reputation. It is usually a very simple matter to verify and correct misinformation posted to this site. That being said, I further agree with Sergey that the list has rules governing participation that should be observed and enforced.
} John A. Robson } _____________________________________________________ } } Boehringer Ingelheim Pharmaceuticals, Inc. } Research and Development } 900 Ridgebury Road / P. O. Box 368 } Ridgefield, CT 06877-0368 } } phone: 203.798.5640 } fax: 203.798.5698 } email: jrobson-at-rdg.boehringer-ingelheim.com } } } } } -----Original Message----- } From: Mike Bode [SMTP:mb-at-Soft-Imaging.com] } Sent: Friday, May 03, 2002 3:05 PM } To: 'Microscopy-at-MSA.Microscopy.Com' } Subject: RE:RONTEC USA Inc., Correction } } ------------------------------------------------------------------------ } 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 } -----------------------------------------------------------------------. } } } Unfortunately that is the case. Someone posts damaging material on this } (or } any other) list, it get's sent around to some people a few times, and } suddenly it is "the official opinion of the microscopy specialists". I am } sure that can do substantial damage. } } And it's not limited to the web or list servers. Audi (the German car } manufacturer) had a good business going in the US until someone decided to } start the engine and put it in forward (or backwards, I don't remember) } and } run the car into a wall. There was a flaw, that allowed users to put the } car } in gear without stepping on the brakes. Although that definitely was a } flaw, } it was blown out of proportion and almost killed the Audi business in the } US. It took them 10 years to get their reputation back, even though I } would } not consider this as dangerous as the tire problem that Firestone/Ford was } experiencing last year. } } Bottom line: Everybody should be careful and check their sources when } posting potentially dmaging material on the listserver. } } But that's just my 2 cents as a vendor. } } mike } } } } } } } } } } } } WE HAVE MOVED { { { { { { { { { } please make a note of the new address below } } Michael Bode, Ph.D. } Soft Imaging System Corp. } 12596 West Bayaud Avenue } Suite 300 } Lakewood, CO 80228 } =================================== } phone: (888) FIND SIS } (303) 234-9270 } fax: (303) 234-9271 } email: mailto:info-at-soft-imaging.com } web: http://www.soft-imaging.com } =================================== } } } } -----Original Message----- } } From: Sergey Ryazantsev [mailto:sryazant-at-ucla.edu] } Sent: Friday, May 03, 2002 6:40 AM } To: Microscopy-at-sparc5.microscopy.com } Subject: Re: RONTEC USA Inc., Correction } } } ------------------------------------------------------------------------ } 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 } -----------------------------------------------------------------------. } } } It's strange to see that one anonymous message could make so much damage } to } the company. It seems to me that reputation of the company depends more } on } the quality of the products/service etc nor on the one anonymous } opinion. From another hand, I think, this ListServer mostly is a place } for } 'customers' to exchange not only scientific ideas but to help each other } to } survive in this 'capitalistic' world. Information about wrongdoing may } help others do not make similar mistake or spend money on bad quality } product/service. This is sort of our 'protection' against bad quality } service/products providers. Again, single decision even published here } could not damage the reputation of the good company with long well } established record of the service to EM community. I know, there are } places on the Internet where you could leave your opinion about some } particular business/company - it's perfectly legal and many institutions } used that lists for decision making. This discussion is more about ethics } } - we all agree that we have rights openly speak here and others have the } rights to know who is speaking. } } Sergey spoke. } } At 02:15 AM 5/3/02, you wrote: } } ------------------------------------------------------------------------ } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } } On-Line Help } } {http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html} http://www.m } sa } .microscopy.com/MicroscopyListserver/FAQ.html } } -----------------------------------------------------------------------. } } } } To the Microscopy & Microanalysis community } } } } Ref.: Anonymous Message posted April 30, } } Subj: RÖNTEC USA Closes Down Operation } } } } Ladies and Gentlemen: } } } } Without any doubt, the Microscopy ListServer is a great facility for the } } Microscopy&Microanalysis community to distribute and exchange useful } } information in a very efficient way and everyone involved in initiation } } and maintenance of this forum highly deserves our community's credit. } } } } However, it appears that at the same time this platform is a quite } } powerful tool for anyone with hostile and bad enough intents to defame } and } } defile disliked entities. This is what we had to learn when the } } unwarranted message regarding an alleged close down of RÖNTEC USA, Inc. } } was spread. It also appears that there is no way to avoid such unfounded, } } } false and misleading information to be posted at the ListServer other } than } } the commitment of all users to the "General Ground Rules on using the } } Microscopy Listserver/Mailreflector" (see msa website), clearly a code of } } } honor. Whatever individual or organization posted this message in their } } malicious attempt of damaging our company and good reputation violated } all } } those general ground rules. May everyone draw his/her own conclusions } } concerning the nature of the information and the integrity of the sender. } } } } We may be allowed to correct the above-mentioned statements about RÖNTEC } } USA, Inc. as follows: 1. There are no plans whatsoever to cease the } } business of RÖNTEC USA, Inc. } } 2. The RÖNTEC Group of companies - like so many others - has not } } remained unaffected by the overall downturn we saw in the economy during } } the year 2001. The situation within our group forced us to implement a } } restructuring program in order to reduce operational costs (as was the } } case throughout the industry - we believe we are in good company here). } } This program was comprising all members of our group, including RONTEC } } USA. The goal was not to cease business, but exactly the opposite - to } } ensure its continuation, in the best interest of our customers. } } 3. Our joint efforts have been successful. The fact is RÖNTEC USA, } } Inc. has had its best sales year since the company's founding in 1999 } } nearly doubling its revenue over the previous year. Why, after having } } worked very hard indeed to get things going and after having eventually } } accomplished that stage, should we consider to discontinue the business? } } Apparently there exists someone or some company who is attempting to } } damage our reputation. Be assured that RÖNTEC USA is in a better position } } } than ever before and will continue to grow and continue to support its } } customers. } } 4. We have never provided misleading information on the equipment we } } } are offering. How long would we survive in this business if we were to } } make promises we can't keep? Due to our companies policy of verifying any } } } information before disclosing it to the public we earned ourselves a } } reputation as a reliable business partner.5. RÖNTEC USA, Inc. does } } have an SEM for sale, however this has absolutely no bearing on the } } viability of the company. } } } } } } Whoever has any questions or the need for more information on this } subject } } may please contact us directly, by phone or otherwise, in the US or at } our } } German headquarters. We at RÖNTEC take great pride in our products and } } services and we have nothing to hide - in contrast to the sender of that } } unfounded message, who chose not to disclose a name. } } In the future may our community be spared such unwarranted assaults. } } } } } } Thomas Schuelein Paul Smith } } President & CEO President & CEO } } RÖNTEC Holding AG RÖNTEC USA, Inc. } } } } } } {/blockquote} {/x-html} } } _____________________________________ } } Sergey Ryazantsev Ph. D. } Electron Microscopy } UCLA School of Medicine } Department of Biological Chemistry } Box 951737 } Los Angeles, CA 90095-1737 } } Phone: (310) 825-1144 } FAX (departmental): (310) 206-5272 } mailto:sryazant-at-ucla.edu } } } }
-----Ursprungliche Nachricht----- Von: Nestor J. Zaluzec [mailto:zaluzec-at-sparc5.microscopy.com] Gesendet: Tuesday, May 07, 2002 3:03 PM An: NewSub-at-sparc5.microscopy.com Betreff: Welcome to the Microscopy Listserver
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********************************************* This Email contains Important Information about the Microscopy Listserver. Please read it all then SAVE a copy for future reference. - Nestor **************************************** To: NewSub-at-MSA.Microscopy.Com } From: "Nestor J. Zaluzec" {zaluzec-at-microscopy.com}
Hi Peter:
I am very sorry to make you and other friends confused with my question.
Actually, I am just doing the regular AFM, that is, using AFM to get the topography information. It is the z height what you mentioned.
I want to put some images in my presentation. While, as you know, 3-D works better than 2-D if you just want to "show" them. The problem is: different 3-D images have their own Z range. If I want to compare them, I'd better use the same Z range for every image, so that when people look at them, they will have some idea immediately.
This is what I want to do: Keep same Z range for different sample's image. But I failed when I tried to reach it by only changing the Z magnification and offset.
But for lots of papers, which have AFM images included, their images have the constant Z range for all the images. So I just wonder whether some of you did this for your own images, and whether you could help me out about this.
Thank you very much!
Sincerely, Xianglin Li
Center for Advanced Material Department of Chemical Engineering University of Massachusetts, Lowell Xianglin_Li-at-student.uml.edu Tel: 978-934-3411
Center for Advanced Material Department of Chemical Engineering University of Massachusetts, Lowell Xianglin_Li-at-student.uml.edu Tel: 978-934-3411
----- Original Message ----- } From: Peter Tomic {PTomic-at-Anadigics.com}
I am working with 27nm cobalt particles that are weakly ferromagnetic (MS = 95 emu/g, HC = 175 Oe) and am attempting some experiments employing static and dynamic magnetic fields. I am currently using a Philips EM400 TEM and am thinking of also using a JEOL 840 SEM to analyze the aggregated structures formed once the particles are dried onto a substrate. The substrates I am using are carbon grids for the TEM and I am planning to use silicon wafers for SEM. I am unsure of the adhesion of the particles to the substrates, although suspect adhesion to the carbon grid will be better than to the silicon (the particles are coated with an organic surfactant). I would prefer to obtain the SEM images without coating the sample. What is the possibility that these particles will be picked up by the lenses in the EM? Are there other considerations I should keep in mind while planning these experiments?
Thank you,
Steve Tripp
Dept. of Chemistry Purdue University West Lafayette, IN 47907
In the early days of materials ultramicrotomy at my laboratory, we plastered more than a few sections of steel onto the polepiece of our EM400T as soon as the polepiece was activated in going from low mag to regular mode. One minute they were there, then---poof! However in an old warhorse like that, there was no noticeable effect on the TEM's performance. (Our superconscientious tech did glare rather strongly just at the thought of such an indiscretion, mind).
So I wouldn't worry too much. We got tired of losing metal thin sections that were dried onto grids in any event, and found that collecting them on the film side of a coated grid resulted in more than enough 'stick' to hold them there. Of course, these sections had pretty huge aspect ratios (thickness/width of several hundred) compared to a particle, but I think your low mass should help out there.
Good luck.
Tom
Dr. Tom Malis Group Leader - Characterization Materials Technology Laboratory Natural Resources Canada (Govt. of Canada) 568 Booth St., Ottawa, Canada K1A 0G1
ph. 613-992-2310 FAX 613-992-8735
email: malis-at-nrcan.gc.ca (currently on assignment as Science Advisor to DG/MTB, can be reached at 613-995-7358, same email)
} ---------- } From: Steven L. Tripp } Sent: Tuesday, May 07, 2002 1:14 PM } To: Microscopy-at-sparc5.microscopy.com } Subject: EM of magnetic particles } } ------------------------------------------------------------------------ } 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 working with 27nm cobalt particles that are weakly ferromagnetic (MS } = } 95 emu/g, HC = 175 Oe) and am attempting some experiments employing static } and dynamic magnetic fields. I am currently using a Philips EM400 TEM and } am thinking of also using a JEOL 840 SEM to analyze the aggregated } structures formed once the particles are dried onto a substrate. The } substrates I am using are carbon grids for the TEM and I am planning to } use } silicon wafers for SEM. I am unsure of the adhesion of the particles to } the } substrates, although suspect adhesion to the carbon grid will be better } than } to the silicon (the particles are coated with an organic surfactant). I } would prefer to obtain the SEM images without coating the sample. What is } the possibility that these particles will be picked up by the lenses in } the } EM? Are there other considerations I should keep in mind while planning } these experiments? } } } Thank you, } } Steve Tripp } } Dept. of Chemistry } Purdue University } West Lafayette, IN 47907 } } }
Yuck I've scrubbed DP's like that before, Sorry You inherited this mess but they will be amazed at how good it works when you are done. yearly PM's are well worth never having to do this again I'm sure you will agree by the time you get it all put back together. Good Luck.
Kathy Napolitano
-----Original Message----- } From: Rosemary White [mailto:rosemary.white-at-csiro.au] Sent: Monday, May 06, 2002 11:43 PM To: ars-at-sem.com Cc: Microscopy-at-sparc5.microscopy.com
Dear Allen,
Yes, well this is the state the instrument was in when I arrived here 2 years ago, but was told "it's OK, it works fine, don't worry about the oil on the viewing window". As the new kid on the block and with no experience in EM maintenance, I found it hard to argue for this full overhaul. And yes, you could get OK images from it, but I still worried about the oil, so finally we are doing something about it.
The diff pumps are out now, and if any of you have looked at Fig. 5.15 in Wilbur Bigelow's Vacuum Methods book you'll have an idea what their innards looked like. The top pump had a little oil left in it, with big chunks of black goop in - and it looks like some of this junk and oil has gone further up the vacuum system. The hot parts had brown to black carbonised oil burnt firmly onto the surface. The innards of the bottom diff pump were coated in what looked like blackstrap molasses - what's left of the original oil, I guess. There was less carbonisation than in the top pump.
So, we're in for a long session, by the looks.......
Thanks again to everyone for suggestions and comments.
cheers, Rosemary
} Rosemary, you've got a lot of 'xplaining to do. } } Has this instrument had any service at all in all those years? These } instruments can be remarkable tolerant, especially if the proper supplies } are used such as a DP oil that will form a non-conductive film. However, } you have two choices - either make column cleanliness a regular affair } where small amounts of contamination are removed at regular intervals, or } make column cleanliness a rare but substantial affair where it is left } alone until a problem develops and a major cleaning is required. } } I have some sympathy for the task you now have, but take solace in the fact } that you brought it upon yourself. What you have is one of the most } sensitive and sophisticated scientific instruments ever made. Treat it in } the future as the fine instrument it is and you will have many more years } of happy service from it. } } Allen R. Sampson } Advanced Research Systems } 317 North 4th. Street } St. Charles, Illinois 60174 } } phone (630) 513-7093 fax (630) 513-7092 http://www.sem.com
Rosemary White Microscopy Centre CSIRO Plant Industry GPO Box 1600 Canberra, ACT 2601 Australia
61- 2 6246 5475 or 61- 0402 835 973 rosemary.white-at-csiro.au
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Hi. We're investigating various alternatives for the polishing of rocks of various kinds. One of the suggestions is to go the Struers' MD-system route, but as you can imagine this is the expensive option. Is there anyone out there using this and how is it working for you? My particular concerns are lif time of the discs and enbedding of foreign particles (mineral frags that may chip off) into the polymer surface rendering these unusable. Thanks, Malc.
-- Dr MP Roberts Phone: [+27](0)46 603 8313 Dept of Geology Fax: [+27](0)46 622 9715 Rhodes University Cell: 083 4060 262 (try your luck!) 6140 Grahamstown e-mail: m.roberts-at-ru.ac.za SOUTH AFRICA
Common sense is (as always) most important. However, as most common sense comes with hindsight I'll give a few thoughts.
I'll assume that you are not thinking of applying fields in-situ or looking for magnetic contrast but if you are there are other considerations.
Don't forget that unless you have a low field pole piece the specimen will be sitting in a field when you analyse it. In the TEM this will be a high field and may negate your ex-situ experiment.
It seems sensible to use a long working distance in the SEM to reduce the field but I have no idea what a SEM field profile looks like.
In the TEM switch off the objective lens before inserting the specimen and slowly increase the strength to avoid sudden field changes.
Even if using a low field pole piece don't forget the return path of the lens field is through the outer column and there will be a high field as the specimen is inserted through the airlock.
Keep your beam current low to prevent the possibility of particle charging adding to the force to free the particles from the substrate.
Don't forget to tap the specimens to free any loose particles before inserting them into the microscope.
Check particle dispersion under an optical microscope first, large agglomerations are more likely to give problems. (You may not see the particles but you will see large agglomerations of particles.)
Good luck, Ron
On Tue, 7 May 2002 12:14:14 -0500 "Steven L. Tripp" {tripp-at-purdue.edu} wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } I am working with 27nm cobalt particles that are weakly ferromagnetic (MS = } 95 emu/g, HC = 175 Oe) and am attempting some experiments employing static } and dynamic magnetic fields. I am currently using a Philips EM400 TEM and } am thinking of also using a JEOL 840 SEM to analyze the aggregated } structures formed once the particles are dried onto a substrate. The } substrates I am using are carbon grids for the TEM and I am planning to use } silicon wafers for SEM. I am unsure of the adhesion of the particles to the } substrates, although suspect adhesion to the carbon grid will be better than } to the silicon (the particles are coated with an organic surfactant). I } would prefer to obtain the SEM images without coating the sample. What is } the possibility that these particles will be picked up by the lenses in the } EM? Are there other considerations I should keep in mind while planning } these experiments? } } } Thank you, } } Steve Tripp } } Dept. of Chemistry } Purdue University } West Lafayette, IN 47907 } } }
---------------------- Mr. R.C. Doole Department of Materials, University of Oxford. Parks Road, Oxford. OX1 3PH. UK. Phone +44 (0) 1865 273701 Fax +44 (0) 1865 283333 ron.doole-at-materials.ox.ac.uk
Dear all, What programs are people using these days for calculating the line direction of dislocations and other linear features (and thus also habit planes of planar features) from measurements made on conventional TEM diffraction contrast images?
Several years ago I did this with Diffract (for Mac) as a PhD student, but no error was included in the analysis, and Diffract was always prone to unexpected crashes. Maybe this is done better in Desktop Microscopist (the successor to Diffract) but I don't know myself.
Or maybe there's some other program to recommend?
I remember seeing a routine published by Fu-Rong Chen and Alex King for Hexagonal Materials which calculated a best fit to available data. Did anyone make such a thing into a program? I could probably do it with Excel, but if somebody has already done it then it saves the work.
Would there be a problem in elevating your samples above the Fermi Temperature and thereby make them non-magnetic? Or would this change the characteristics of your alloy? I am interested since I have had a similar problem with an iron alloy but solved it by coating and imaging as you have mentioned.
With respect to these particles on a Si wafer in SEM, you may try depositing Si3n4 [silicon nitride] over the particles while on the wafer if you have access to a deposition system such as a PECVD. This can be a very thin film, just a few hundred angstroms, but it will lock these particles to the surface and still allow imaging even if they are irregular surfaces.
Peter Tomic Anadigics, Inc.
-----Original Message----- } From: Steven L. Tripp [mailto:tripp-at-purdue.edu] Sent: Tuesday, May 07, 2002 1:14 PM To: Microscopy-at-sparc5.microscopy.com
I am working with 27nm cobalt particles that are weakly ferromagnetic (MS = 95 emu/g, HC = 175 Oe) and am attempting some experiments employing static and dynamic magnetic fields. I am currently using a Philips EM400 TEM and am thinking of also using a JEOL 840 SEM to analyze the aggregated structures formed once the particles are dried onto a substrate. The substrates I am using are carbon grids for the TEM and I am planning to use silicon wafers for SEM. I am unsure of the adhesion of the particles to the substrates, although suspect adhesion to the carbon grid will be better than to the silicon (the particles are coated with an organic surfactant). I would prefer to obtain the SEM images without coating the sample. What is the possibility that these particles will be picked up by the lenses in the EM? Are there other considerations I should keep in mind while planning these experiments?
Thank you,
Steve Tripp
Dept. of Chemistry Purdue University West Lafayette, IN 47907
I was wondering if the group had any wisdom to impart that could help me with my particle analysis work. I'm trying to analyse stack effluent collected on polycarbonate filters during an airborne survey. I'm using WDS because the sample contain Pb and S. The particles range from less than one to ~ 10 um. My problem is that most of the are charging and therefore the beam is drifting off of them during the course of analysis. The samples polycarbonate filtres are attached to Al stubs using double stick carbon and heavily carbon coated while on a planetary rotating table. I'm using 15 kV (I need to see Fe)and 10-20 nA current. I've had some success overscanning the particles (i.e analysing with a raster that is the same size as the particle) but some of the larger particles are multiphase and i would like to use a smaller beam to determine their chemistry. Any tips or comments from people with experience in this type of work would be gladly accepted.
Thanks
Glenn Glenn Poirier Microbeam Specialist
Mine and Mineral Science Laboratories (CANMET) Rm. 213b, 555 Booth st. Ottawa, On, K1A 0G1 TEL: (613) 947-9833 glpoirie-at-nrcan.gc.ca
In the below first paragraph below I mentioned "Fermi Temperature" and should have said "Curie Temp."
My appologies.
Peter
-----Original Message----- } From: Peter Tomic [mailto:PTomic-at-anadigics.com] Sent: Wednesday, May 08, 2002 8:44 AM To: 'Steven L. Tripp'; Microscopy-at-sparc5.microscopy.com
Steve;
Would there be a problem in elevating your samples above the Fermi Temperature and thereby make them non-magnetic? Or would this change the characteristics of your alloy? I am interested since I have had a similar problem with an iron alloy but solved it by coating and imaging as you have mentioned.
With respect to these particles on a Si wafer in SEM, you may try depositing Si3n4 [silicon nitride] over the particles while on the wafer if you have access to a deposition system such as a PECVD. This can be a very thin film, just a few hundred angstroms, but it will lock these particles to the surface and still allow imaging even if they are irregular surfaces.
Peter Tomic Anadigics, Inc.
-----Original Message----- } From: Steven L. Tripp [mailto:tripp-at-purdue.edu] Sent: Tuesday, May 07, 2002 1:14 PM To: Microscopy-at-sparc5.microscopy.com
I am working with 27nm cobalt particles that are weakly ferromagnetic (MS = 95 emu/g, HC = 175 Oe) and am attempting some experiments employing static and dynamic magnetic fields. I am currently using a Philips EM400 TEM and am thinking of also using a JEOL 840 SEM to analyze the aggregated structures formed once the particles are dried onto a substrate. The substrates I am using are carbon grids for the TEM and I am planning to use silicon wafers for SEM. I am unsure of the adhesion of the particles to the substrates, although suspect adhesion to the carbon grid will be better than to the silicon (the particles are coated with an organic surfactant). I would prefer to obtain the SEM images without coating the sample. What is the possibility that these particles will be picked up by the lenses in the EM? Are there other considerations I should keep in mind while planning these experiments?
Thank you,
Steve Tripp
Dept. of Chemistry Purdue University West Lafayette, IN 47907
We sold uranyl formate for many years but we discontinued it in 1995 and have been unable to find a new source.
John Arnott --
**** Please Note Our New Address, Fax and Phone Numbers ****
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John Hoffpauir 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 } -----------------------------------------------------------------------.} } can anyone tell me where i might purchase uranyl formate in the US?
John Hoffpauir wrote: ================================================== can anyone tell me where i might purchase uranyl formate in the US? ================================================== Try URL http://www.2spi.com/catalog/chem/stain.shtml
The product is in stock.
Chuck
Disclaimer: SPI Supplies is a supplier of uranyl formate.
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We need to replace a Nikon Condenser Lens (MBL12100-AL1) from a Nikon Phase Contrast Unit (1.25 59842) being used on a Nikon Labophot Microscope. This microscope is being used for the phase contrast analysis of air samples for fiber concentration.
We have been in touch with Nikon and one of their suppliers but so far without too much success. Does anyone know of any other sources for this lens or a replacement phase contrast unit?
Thanks .
Stanley H. Gelles Principal Scientist CC Technologies 6141 Avery Road Columbus, OH 43220 614-761-1214 FAX 614761-1633 sgelles-at-cctlabs.com
Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (alm958-at-lulu.it.northwestern.edu) from http://www.msa.microscopy.com/Ask-A-Microscopist.html on Wednesday, May 8, 2002 at 17:58:01 ---------------------------------------------------------------------------
Email: alm958-at-lulu.it.northwestern.edu Name: Tony Meier
Organization: Northwestern University
Education: Graduate College
Location: Evanston, IL ,USA
Question: Why are we getting a clear and focused image with our infinity corrected objective attached directly to our vidicon camera, without using a tube lens? I realize that we are not getting anywhere near the 10x mag of the objective but I don't understand why we are getting an image at all since we are not forming a real image on our cameras sensor.
I am looking to purchase a fluorescent microscope ( I am partial to Olympus and Leica but am open to other options). It needs to have oil (100X) and phase contrast for LM, DIC would be nice too, and all three filter sets, DAPI, FITC, and TRITC. A used one in good condition would be acceptable.
Dr.Tina S. Schwach, President Microscopy Consulting Services Inc. 651-681-0112
I am interested in the current negative-scanner technology, but I would like to find a non-contact scanner. EM emulsions are very soft and very high resolution, so since these negatives represent the basis for long term archiving, I wouldn't want to sacrifice microscopic information by placing it on a surface of glass (or any surface) with potentially damaging particulate on the surface. Even projection holders for Negatives have no glass that contact the emulsion. So what is the current negative scanner technology?? Non-contact..?
During several years I used Ralph Knifes to section Glycol Methacrylate embedded material (2-3 micrometer) for LM. Has anyone experience in sectioning with disposable blades?
Many of our customers are using Microtek Artixscan 2500 and 1100 scanners as well as their mechanical twins, the Agfa Duoscan T2500 and Hi-D. Agfa has discontinued the Duoscan line but the Microteks are still available. The 2500 has higher optical resolution, the 1100 has a wider dynamic range. These scanners hold films in a glassless drawer much like a negative carrier in an enlarger. Most are using the 4x5 opening to hold the 3.25 x 4 EM negs.
More information is available at http://www.microtekusa.com/as2500.html for the 2500, and http://www.microtekusa.com/as1100.html for the 1100. We also have a PDF available.
George
George Laing National Graphic Supply ph 800.223.7130 x3109 f 800.832.2205 email scisales-at-ngscorp.com
} I am interested in the current negative-scanner } technology, but I would like to find a non-contact } scanner.
Life Science Research Assistant (LSRAI) (HR #001178). Range: 2P1.
DESCRIPTION: Life Sciences Research Assistant is sought for day to day managing of the Cell Sciences Imaging Facility (CSIF). The CSIF is a service center that specializes in the use of high technology fluorescent microscopes (confocal, deconvolution, ratio imaging) in biomedical research. LSRA duties include: training users in operation of microscopes, providing ongoing technical supervision, performing routine maintenance/cleaning and arranging for service of microscopes and computers. Additionally, LSRA will provide some administrative support such as assisting in setting up user accounts, updating user databases and monthly billing routines.
All of CSIF microscopes are interfaced with computers for data collection and analysis. Basic knowledge of operating systems (Windows, Mac, Unix ), graphics programs (PhotoShop, Illustrator) and general computer usage (transfer of files between platforms, file format differences) is essential. LSRA should understand optical properties of fluorescence. Preference will be given to applicants who have both basic microscopy and computer experience, but a willingness to learn is key. Qualifications: BS degree required, as well as good communication skills, patience, and the ability to work independently. Good problem solving skills are essential. This is a great opportunity learn state-of-the-art technology and be exposed to current biomedical research.
Salary range $37,100 - 41,000, depending upon experience. There is no relocation assistance; position is available immediately. Please send resume directly to:
Jon Mulholland, Director Cell Sciences Imaging Facility Beckman Center B050 Stanford University School of Medicine Stanford, CA 94305
I am looking to obtain a pore size distribution and a porosity estimate of a sample from two scanning electron micrographs taken at a 10° offset from one another. Both files are tiff format. All of the software I was able to find uses z-stacking and not an angular offset. Does anyone have any recommendations on software for generating a 3-D image and obtaining the information? Thank you for your time.
Dan
**************************************************************************** ****************************************************************** Daniel D. Smolko, Ph.D. Senior Research Scientist & BioChemical Engineer Nanogen, Incorporated 10398 Pacific Center Court San Diego, CA 92121
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We have a visiting scientist interested in learning FISH techniques -- are there any class(es)/workshops out there being offered in the near future (ie. this summer or fall)?
TIA,
John
John W. Mattila Iowa State University Bessey Microscopy Facility Room 1, Bessey Hall Ames, IA 50011-1020
Hi Malc, We polish many different crystals and materials here. We also build our own lapping and polishing equipment. I thought I might be able to assist you in making a cost-effective choice in selecting equipment if I were able to learn just exactly what you need to do. We routinely achieve surfaces with as low as 3 to 4 Angstrom RMS roughness here. Let me know if I can be of help to you.
Cheers, Michael Urbanik } From the U.S.A., the keeper of the Flame of Freedom. www.crystalguru.com
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
} Hi. } We're investigating various alternatives for the polishing of rocks } of various kinds. One of the suggestions is to go the Struers' MD-system } route, but as you can imagine this is the expensive option. Is there } anyone out there using this and how is it working for you? My particular } concerns are lif time of the discs and enbedding of foreign particles } (mineral frags that may chip off) into the polymer surface rendering } these unusable. } Thanks, } Malc.
-- Dr MP Roberts Phone: [+27](0)46 603 8313 Dept of Geology Fax: [+27](0)46 622 9715 Rhodes University Cell: 083 4060 262 (try your luck!) 6140 Grahamstown e-mail: m.roberts-at-ru.ac.za SOUTH AFRICA
Dan You may find the Soft Imaging System web site relevant. There is a module for AnalySIS that calculates quantitative elevation maps based on stereo pair images
----- Original Message ----- } From: "Smolko, Dan" {DSmolko-at-Nanogen.com} To: "'Microscopy-at-MSA.Microscopy.Com'" {Microscopy-at-sparc5.microscopy.com} Sent: Thursday, May 09, 2002 6:21 PM
To all subscribers:
I am looking to obtain a pore size distribution and a porosity estimate of a sample from two scanning electron micrographs taken at a 10° offset from one another. Both files are tiff format. All of the software I was able to find uses z-stacking and not an angular offset. Does anyone have any recommendations on software for generating a 3-D image and obtaining the information? Thank you for your time.
Dan
********************************************************************** ****** ****************************************************************** Daniel D. Smolko, Ph.D. Senior Research Scientist & BioChemical Engineer Nanogen, Incorporated 10398 Pacific Center Court San Diego, CA 92121
|||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||| |||||| |||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||| |||||| ||||||||||||||||||||||||||||| This e-mail message is intended only for use by the individual, or recipient(s) entity to which it is addressed. This message is confidential and may contain information that is privileged, confidential and is exempt from disclosure under applicable law. If you are not the intended recipient(s), you may not review, copy, or distribute this message. If you have received this communication in error, please notify us immediately by e-mail, or telephone and delete the original message. Thank you. |||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||| |||||| |||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||| |||||| |||||||||||||||||||||||||||||
} During several years I used Ralph Knifes to section Glycol Methacrylate } embedded material (2-3 micrometer) for LM. } Has anyone experience in sectioning with disposable blades? } } Thanks for the courtesy } Bruno Dore
Bruno -
You can hand-break Ralph knives from glass microscope slides. They're cheap, good, and disposable.
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
what you are looking for is a stereo reconstruction program. There are several available, we make on too. If you want more information, please contact me offline at the address below.
mike
} } } } } } } } } } WE HAVE MOVED { { { { { { { { { please make a note of the new address below
Michael Bode, Ph.D. Soft Imaging System Corp. 12596 West Bayaud Avenue Suite 300 Lakewood, CO 80228 =================================== phone: (888) FIND SIS (303) 234-9270 fax: (303) 234-9271 email: mailto:info-at-soft-imaging.com web: http://www.soft-imaging.com ===================================
-----Original Message----- } From: Smolko, Dan [mailto:DSmolko-at-Nanogen.com] Sent: Thursday, May 09, 2002 11:21 AM To: 'Microscopy-at-MSA.Microscopy.Com'
To all subscribers:
I am looking to obtain a pore size distribution and a porosity estimate of a sample from two scanning electron micrographs taken at a 10° offset from one another. Both files are tiff format. All of the software I was able to find uses z-stacking and not an angular offset. Does anyone have any recommendations on software for generating a 3-D image and obtaining the information? Thank you for your time.
Dan
**************************************************************************** ****************************************************************** Daniel D. Smolko, Ph.D. Senior Research Scientist & BioChemical Engineer Nanogen, Incorporated 10398 Pacific Center Court San Diego, CA 92121
|||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||| |||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||| ||||||||||||||||||||||||||||| This e-mail message is intended only for use by the individual, or recipient(s) entity to which it is addressed. This message is confidential and may contain information that is privileged, confidential and is exempt from disclosure under applicable law. If you are not the intended recipient(s), you may not review, copy, or distribute this message. If you have received this communication in error, please notify us immediately by e-mail, or telephone and delete the original message. Thank you. |||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||| |||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||| |||||||||||||||||||||||||||||
in addition to the SIS stereo reconstruction module, there is a similar routine that is part of Fovea Pro. See http://ReindeerGraphics.com/foveapro2/surface.html
Timothy G. Schneider Director of Electron Microscopy Department of Pathology Thomas Jefferson University Room 229 JAH 1020 Locust Street Philadelphia Pa. 19107 215-503-4798 work 610-613-8170 cell Timothy.Schneider-at-Mail.TJU.edu
We have a Philips EM400T in our lab. It is old but still works well. However, I noticed that illumination can be observed as soon as High Tension is on. As a result, the saturation point is very low, only two or three steps of filament current. My question is why there is a clear emmission current without any filament current? Is this caused by a gun fault? What can we do about it? Thank you very much in advance!
Yanling
Dr.Y.L.Chen MicroStructural Studies Unit School of Engineering The University of Surrey Guildford, Surrey GU2 7XH, England
--------------------------------------------- This message was sent using UNIS MailSystem.
} } I am interested in the current negative-scanner } } technology, but I would like to find a non-contact } } scanner.
If you have a robust budget, (12-18K$) you might check the Imacon scanners, either the Flextite 848 or Precision III.
I have no commercial interest in these products. -- Gary P. Radice gradice-at-richmond.edu Associate Professor of Biology 804 289 8107 (voice) University of Richmond 804 289 8233 (FAX) Richmond VA 23173 http://www.science.richmond.edu/~radice
I am looking for individuals who are willing to review and write a reviewed article of the following books for the MSA Journal.
1. "Electron Microscopy and Analysis 2001" (A materials related book). Edited by M. Aindow and C.J. Kiely 2. "Luminescence Biotechnology Instruments and Applications" Edited by Knox Van Dyke, Christopher Van Dyke and Karen Woodfork 3. " Photography with a Microscope" Fred Rost and Ron Oldfield 4. " Selected Papers on Optical Low-Coherence Reflectometry & Tomography" Edited by Barry R. Masters 5. "Near-Infrared Technology in the Agricultural and Food Industries" Edited by Phil Williams and Karl Norris
If you are interested in participating please send me the title of the book you would like to review and it will be sent to you ASAP. Selection will be make on a first come first serve basis.
Thank you!
JoAn Hudson, PhD. Institute of Neuroscience 222 Huestis Hall University of Oregon, Eugene, OR 97403
Please find enclosed deadlines related to TNT2002 conference to be held in Santiago de Compostela (Spain): September 9-13, 2002:
!!May 17, 2002: Extended "Graduate grant request" deadline!! !!May 24, 2002: Extended Abstract submission deadline!! June 03, 2002: Notification to the authors by e-mail of the accepted papers for oral presentation or poster / Notification of graduate travel awards June 17, 2002: Registration deadline July 01, 2002: Preliminary programme July 15, 2002: Final programme & "Extended Abstracts" booklet printing September 09, 2002: Manuscript submission deadline (to be published in "Nanotechnology" journal)
40 Grants for students are available: 20 for US and 20 for Europe - please check http://www.cmp-cientifica.com/cientifica/frameworks/generic/public_users/TNT02/TNT02_grants.html for more info.
If you are interested in presenting an oral contribution, please send me (mailto:antonio-at-cmp-cientifica.com) as soon as possible a tentative title talk and an extended abstract (2 pages max including figures) - only a few slots are still available. Therefore, the committee will select papers for oral presentation and we will notify authors shortly. We encourage participants to present posters during TNT2002.
If you need more information, please do not hesitate to contact me. If you accept this invitation, please respond by email as soon as possible.
Hoping to receive a positive answer to our invitation.
Antonio Correia
----------------------------------------------------------------------------------- Dr. Antonio CORREIA - Coordinator of the IST Nanoelectronics Network (PHANTOMS) CMP Cientifica S.L. Phone: +34 91 6407187 Fax: +34 91 6407186 mailto:antonio-at-cmp-cientifica.com WEB site: http://www.cmp-cientifica.com/ PHANTOMS WEB site: http://www.phantomsnet.com/ TNT2002: http://www.cmp-cientifica.com/TNT2002.html
1. Masakasu Aono (Riken, Japan) 2. Phaedon Avouris (IBM, USA) 3. Yoshio Bando - National Institute for Materials Science (NIMS) (Japan) 4. Flemming Besenbacher (Aarhus University, Denmark) 5. Mark Blamire (University of Cambridge, UK) 6. Guillermo Bozzolo (NASA Glenn Research Center, USA) 7. George Bourianoff (Intel, USA) 8. Roberto Car (Princeton University, USA) 9. Ignacio Cirac (Max-Planck Institut fur Quantenoptik, Germany) 10. Dongmin Chen (Rowland Institute for Science, Cambridge, MA, USA) 11. Wonbong Choi (Samsung, Korea) 12. Harold Craighead (Cornell University, USA) 13. Supriyo Datta (Purdue University, USA) 14. Cees Dekker (Delft University, Netherlands) 15. Pedro Echenique (Donostia International Physics Center (DIPC), Spain) 16. Andreas Engel (Basel University, Switzerland) 17. Leo Esaki (Shibaura Institute of Technology, Japan) - Invited Lecture 18. Fernando Flores (Universidad Autonoma de Madrid, Spain) 19. Harald Fuchs (Munster University, Germany) 20. Christoph Gerber (IBM, Switzerland) 21. James Gimzewski (UCLA, USA) 22. Herb Goronkin (Physical Research Laboratory - Motorola Labs, USA) 23. Masahiko Hara (Tokyo Institute of Technology, Japan) 24. James Heath (UCLA, USA) 25. Kikuji Hirose (Osaka University, Japan) 26. Christian Joachim (CEMES/CNRS, France) 27. Sajeev John (University of Toronto, Canada) 28. Dieter Kern (Tuebingen University, Germany) 29. Uzi Landman (Georgia Institute of Technology, USA) 30. Stuart Lindsay (Arizona State University, USA) 31. Daniel Loss (Basel University, Switzerland) 32. Ramesh G. Mani (Harvard University, USA) 33. Meyya Meyyappan (NASA, USA) 34. Seizo Morita (Osaka University, Japan) 35. Rodolfo Miranda (Universidad Autónoma de Madrid, Spain) 36. Gernot Pomrenke (Air Force Office of Scientific Research, USA) 37. Calvin Quate (Stanford University, USA) 38. Jan van Ruitenbeek (Leiden University, Netherlands) 39. Lars Samuelson (Lund University, Sweden) 40. Christian Schoenenberger (Basel University, Switzerland) 41. Ivan Schuller (University of California, USA) 42. Clivia Sotomayor Torres (Wuppertal University, Germany) 43. Shen Tsai (NEC Fundamental Research Laboratories, Japan) 44. Christian Urbina (CEA-Saclay, France) 45. Luis Vina (Universidad Autonoma de Madrid, Spain) 46. Mark Welland (University of Cambridge, UK) 47. Stanley Williams (HP, USA)
I have come across a Gatan model 628/2 single tilt hot stage (1300C) and heating control unit that was purchased for a Hitachi H600 100Kv TEM but was never used. It was apparently tucked away in the lab by my predecessor immediately after its purchase and was recently discovered after having already replaced this microscope. I would like to know if anyone with a similar microscope is interested in actually using it.
Please contact me off-line to discuss in more detail.
George R. Munzing Jr. Engelhard Corporation 25 Middlesex-Essex Tpk. Iselin, NJ 08830 TELE 732-205-7030 FAX 732-205-5300
I would appreciate hearing from people taking color digital images. Is there another slide presentation software, other than Powerpoint, that one can use to show histology or fluorescence micrographs in a lecture or meeting. The problem is pasting high resolution images to a Powerpoint slide - quite often we have to reduce the size or the resolution of the images and the images appear washed out. It defeats the purpose of using high resolution cameras to capture images. Any comments/suggestions/recommendations would be greatly appreciated.
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
At 06:24 AM 5/10/02, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
_____________________________________
Sergey Ryazantsev Ph. D. Electron Microscopy UCLA School of Medicine Department of Biological Chemistry Box 951737 Los Angeles, CA 90095-1737
If you need some program just to show already prepared images (slide show) you may try InfanView - this freeware software were discussed recently on ListServer and received very high marks. Again, it's only for demonstration, you may not create PowerPoint-like presentation in it. You may show already prepared (even in Powerpoint I believe, not sure) images. It's very good 'viewer'. It has some very nice features like - it may shrink your image to the screen size and it's so quick. I am using it to show my EM pictures 20-50 Mb in size... http://www.irfanview.com/ Sergey
At 12:22 PM 5/10/02, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
_____________________________________
Sergey Ryazantsev Ph. D. Electron Microscopy UCLA School of Medicine Department of Biological Chemistry Box 951737 Los Angeles, CA 90095-1737
I would wager that the problem isn't with PowerPoint, but rather the projector. Consider that most of the projectors in use now are 1024 x 728 pixels. The whole PowerPoint slide takes that up. If your slide in PowerPoint is set up for 10" x 7.5" (the default) and your image is put on the slide as a 4"x5", then whatever resolution your image was taken at is still only projected at 512x364 pixels.
Now consider using overheads -still not the best, but let's say that you have a good printer that you can print at 300 dpi. (Sublimation dye printers can do this and good quality inkjets can come close to doing this with 256 levels per color.) A 4"x5" print on the slide can still have a size of 1200 x 1500 pixels without loosing anything.
Add to this, the problems of projecting the full color range with projectors. I have read about this, but am not qualified to discuss it.
My advice is to stay with overhead transparencies and forget the fancy slide effects that you can do with PowerPoint or other presentation software.
-Scott
Scott D. Walck, Ph.D. PPG Industries, Inc. Glass Technology Center P. O. Box 11472 (letters) Guys Run Rd. (packages) Pittsburgh, PA 15238-0472
Walck-at-PPG.com
(412) 820-8651 (office) (412) 820-8515 (fax)
-----Original Message----- } From: Corazon D. Bucana [mailto:bucana-at-audumla.mdacc.tmc.edu] Sent: Friday, May 10, 2002 3:22 PM To: Microscopy-at-sparc5.microscopy.com
I would appreciate hearing from people taking color digital images. Is there another slide presentation software, other than Powerpoint, that one can use to show histology or fluorescence micrographs in a lecture or meeting. The problem is pasting high resolution images to a Powerpoint slide - quite often we have to reduce the size or the resolution of the images and the images appear washed out. It defeats the purpose of using high resolution cameras to capture images. Any comments/suggestions/recommendations would be greatly appreciated.
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
You might try using the slideshow function available in Irfanview freeware.
www.irfanview.com
Best,
Angela
----------------------------------------- Angela V. Klaus, Ph.D. Director, Microscopy and Imaging Facility American Museum of Natural History Central Park West at 79th Street New York, NY 10024 USA Email: avklaus-at-amnh.org Tel: 212-769-5977 Fax: 212-496-3480 -----------------------------------------
On Fri, 10 May 2002, Corazon D. Bucana 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 would appreciate hearing from people taking color digital images. Is } there another slide presentation software, other than Powerpoint, that one } can use to show histology or fluorescence micrographs in a lecture or } meeting. The problem is pasting high resolution images to a Powerpoint } slide - quite often we have to reduce the size or the resolution of the } images and the images appear washed out. It defeats the purpose of using } high resolution cameras to capture images. Any } comments/suggestions/recommendations would be greatly appreciated. } } 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 } }
Hi Cora, I've used a piece of software called "UPresent" - its very good for multi-media work, but the last version I used was a little light on text and outlining capabillities. Here is the URL:
http://www.codeblazer.com/products.html
-Brad
---------- From: Corazon D. Bucana Sent: Friday, May 10, 2002 12:22 PM To: Microscopy-at-sparc5.microscopy.com Subject: slide presentation software
------------------------------------------------------------------------ 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 would appreciate hearing from people taking color digital images. Is there another slide presentation software, other than Powerpoint, that one can use to show histology or fluorescence micrographs in a lecture or meeting. The problem is pasting high resolution images to a Powerpoint slide - quite often we have to reduce the size or the resolution of the images and the images appear washed out. It defeats the purpose of using high resolution cameras to capture images. Any comments/suggestions/recommendations would be greatly appreciated.
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
Hi everybody - using a JEOL 5900LV, recently replaced tungsten filament, got great images, few days later image looked like I was in backscatter mode instead of secondary. Stubs were coated 360ang of Au, stubs are flush with sample holder; 20kv, WD 8mm, ss 37 - looking at diatoms 1)aligned gun 2)checked the wobbler Any suggestions of what is going on? Thanks Barb
} From you post, I get the impression that you are reducing the resolution of the image before inserting into Powerpoint. This is one way to make image fit into the slide image area, but does decrease the resolution of the projected image. You can insert the image at full resolution, then size the image on the slide using the Format Image function.
-- Larry D. Hanke, P.E. Materials Evaluation and Engineering, Inc. Practical Solutions Through Technology and Innovation http://www.mee-inc.com (763) 449-8870
I second Scott Walck's comments and add a thought.
The limitation is most likely the projector technology. You are limited to 1024x768 resolution input on the newer projectors. There might still be a question as to whether all that input ends up as output. I have an adapter to take computer input (maybe even up to 1280x1024) and convert it to make it suitable for a video projector. But that projector can only handle NTSC which is a little worse that VGA (640x480) resolution. So all I put in definitely does not make it out there. I also know the color rendition is rather poor.
Scott suggested overheads as an option. I agree and might suggest 35mm slides as another alternative. Our campus has (or at least had) a centralized slide maker that could take Power Point or any printed output and render it at 4000x3000 pixels, IIRC.
But will your audience be able to resolve that much detail from where they are sitting?
I would like to hear from someone who can speak authoritatively on the physiology of the matter. My own sense is that anything more than 1024 pixels across will not be appreciated from normal viewing distance. 1024-pixel images may seem pixelated to someone standing a few feet away from the screen, but I doubt that a viewer sitting in the front row would notice.
For that reason, I take the approach of simply recording multiple images from our SEMs at 1024-pixels across showing the appropriate level of detail in each image. A 40-MB image certainly contains lots of information; however, it can really only be appreciated one 1024-pixel image at a time. I suggest that is the way the presentations will need to be prepared.
At 03:22 PM 5/10/02 -0400, you wrote:
} I would appreciate hearing from people taking color digital images. Is } there another slide presentation software, other than Powerpoint, that one } can use to show histology or fluorescence micrographs in a lecture or } meeting. The problem is pasting high resolution images to a Powerpoint } slide - quite often we have to reduce the size or the resolution of the } images and the images appear washed out. It defeats the purpose of using } high resolution cameras to capture images. Any } comments/suggestions/recommendations would be greatly appreciated. } } 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
------------------------------------------- No files should be attached to this message ------------------------------------------- Warren E. Straszheim, Ph.D. Materials Analysis and Research Lab Iowa State University 23 Town Engineering Ames IA, 50011-3232
I am interested in opinions on how long it takes to prepare a routine chemically fixed, resin embedded biological sample for TEM (by an average technician). I need to work out how many samples could reasonably be prepared by one person in a year.
I am interested in opinions on how long it takes to prepare a routine chemically fixed, resin embedded biological sample for TEM (by an average technician). I need to work out how many samples could reasonably be prepared by one person in a year.
I don't know the 420 but as there have been no other responses maybe I can shed some light on your question.
} From memory, when we had our Philips 300 the filament was always on at a low level, the filament control increased this level but never switched it off. I guess it was interlocked with the vacuum or something, I'm a little hazy about the details. On the back of the console was a switch (I think marked high and low) that would adjust the current setting.
It sounds like your 420 is similar, ie. there is a heating current even though the filament control is off. As soon as you have HT you have emission. It may be that this batch of filaments have slightly thinner wire or that the filament is not set correctly in the Wenhelt. If the filament is set correctly and there is a switch for the filament current that is set on 'high' try setting it to 'low'. If you can still saturate the filament on that setting then that's OK.
Maybe the quiescient current circuit is playing up and giving too high a current?
If that is not the case then I have no idea how you can get a beam without heating unless you have field emission from a very sharp tip on the filament. Not that likely at 120kV but seen at 1MeV on HVEMs.
Good luck, Ron
On Fri, 10 May 2002 14:39:57 GB "Y.Chen-at-surrey.ac.uk"-at-sparc5.microscopy.com wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Dear All, } } We have a Philips EM400T in our lab. It is old but still works well. However, I } noticed that illumination can be observed as soon as High Tension is on. As a } result, the saturation point is very low, only two or three steps of filament } current. My question is why there is a clear emmission current without any } filament current? Is this caused by a gun fault? What can we do about it? } Thank you very much in advance! } } Yanling } } Dr.Y.L.Chen } MicroStructural Studies Unit } School of Engineering } The University of Surrey } Guildford, Surrey } GU2 7XH, England } } } --------------------------------------------- } This message was sent using UNIS MailSystem. } } }
---------------------- Mr. R.C. Doole Department of Materials, University of Oxford. Parks Road, Oxford. OX1 3PH. UK. Phone +44 (0) 1865 273701 Fax +44 (0) 1865 283333 ron.doole-at-materials.ox.ac.uk
Kathy, It'll depend, how much you'll pay for it. If you offer $50-60K, S/he will make a LOT of samples to you!!! There is no 'average' technician in EM. EM is very sophisticated area and in order to have necessary knowledge, experience etc, you have to spend 2-3-5 years. I am not talking about 'hands' - it comes from God. It's not easy to find such qualified person. 'Average' person will kill your most valuable sample in two minutes... Good luck. Sergey
At 03:46 PM 5/13/02 +1000, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Dear Listers, I am looking for programmes (preferably free!)that will enable me to read jpeg files recovered after deletion, or corruption of the file marker. I have tried a few of the better known jpeg file readers without success. Thanks, Jeremy Reply to jb_sanderson-at-yahoo.com
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If you want a scanner for smaller negs(35mm or slides), we have a Nikon Super Coolscan 4000 scanner that does quite well and costs less. I think it cost between 1&2K. Less expensive scanners I've used tend to put lines in the image or have missing pixels.
Karen Pawlowski, Ph.D. Research Scientist UT Dallas
Gary Radice wrote: } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } } I am interested in the current negative-scanner } } } technology, but I would like to find a non-contact } } } scanner. } } If you have a robust budget, (12-18K$) you might check the Imacon } scanners, either the Flextite 848 or Precision III. } } I have no commercial interest in these products. } -- } Gary P. Radice gradice-at-richmond.edu } Associate Professor of Biology 804 289 8107 (voice) } University of Richmond 804 289 8233 (FAX) } Richmond VA 23173 http://www.science.richmond.edu/~radice
Microscopists, Does anyone know of a way (quant. or qualitative) to meause the amount of thickness coating a protein sample with platinum in a metal evaporation run? I don't have a quartz thickness monitor, so is there some extrapolation you can do based on starting and ending material? Right now all we do is use filter paper wedges to estimate shadow thickness (not empirically). Thank you.
Funny you should ask. I wrote a post last night but wasn't going to post it until tomorrow.
In the late 1960s there were charts called nomographs to graphically estimate the thickness of films evaporated onto substrates. They were kind of a graphical slide rule to figure out how much metal to evaporate onto a substrate. I can post a better email from home but this is the link to a nomograph on the web.
The scale at the top is the bulk density of the element or alloy. It is not labeled with the number scale, only the elements. Neither is carbon (near Be), Ge and some alloys like Au-Pd shown.
The formula used for these nomograph charts and converted to use bulk densities is:
wt = [4 * Pi * d˛ * t * rho * (10^-5)]/(sin s)
wt to use is in mgs d is the distance from the point source to the sample target in cms. t is the thickness in angstroms, Ĺ. rho is the bulk density, 21.45 grams per cmł for Pt. 10 EE -5 is to get the units right. s is the shadowing angle measured at the target (as I recall) and that is subtended by the point source and the plane of the sample.
It is easy to derive this formula from surface area concepts and densities.
For straight down evaporations, sin 90ş = 1. The above nomograph doesn't have a scale for shadowing angle. The formula will tell you how to correctly ESTIMATE the amount of material you used.
Hope this helps.
Paul Beauregard Senior Research Associate PPG Industries Monroeville Technical Center Monroeville, PA 15146
-----Original Message----- } From: Mike Delannoy [mailto:delannoy-at-jhmi.edu] Sent: Monday, May 13, 2002 11:20 AM To: microscopylistserver
Microscopists, Does anyone know of a way (quant. or qualitative) to meause the amount of thickness coating a protein sample with platinum in a metal evaporation run? I don't have a quartz thickness monitor, so is there some extrapolation you can do based on starting and ending material? Right now all we do is use filter paper wedges to estimate shadow thickness (not empirically). Thank you.
Is it possible to recover corrupted JPEG file specifically? Never hear about that. I could talk about PC/Win platform only. Windows NT itself (NTFS file system) has internal ability to recover corrupted files (any). It's called 'checkdisk' I believe. It's in the standard Windows package. Similar things should be in win2000. You may also run Norton Disk Doctor on any Win platform - it works great. The things about that: all these programs are not specific to the JPEG files. So, I am not sure how it may help in your particular case. By the way, for PC/Win I would strongly recommend to have Norton Utilities on HD: very useful stuff. Sergey
At 01:16 PM 5/13/02 +0100, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
I'd like to echo Ron's advice regarding checking that the filament is set up correctly in the wehnelt and that it meets the manufacturers specs (thickness, material, etc). The type of problem you described can be caused by any number of faults in the HT circuitry of your 400T, but your first and most likely source, and easiest and least expensive to fix, would be a filament exchange. If that doesn't cure your problem I would recommend having a qualified service engineer in to analyse the situation. We once had a similar problem on our CM12 (which has a nearly identical HT set) and after cleaning the emission chamber, cleaning then replacing the gun, and just before exchanging the HT generator tank, we were able to prove that our cable was breaking down at voltages greater than 40KV. This created all kinds of bias problems which manifested with the symptoms you have described. When the problem first started occurring, it was suspected that we had a malfunction in the emission section of our HT tank. The filaments could be set very far back in the wehnelt assembly to achieve somewhat "normal" heating and illumination behaviour, but changing the Emission setting then had negligible impact on beam current. If these symptoms are what you are noticing with your TEM, you might want to check the HT cable. This is probably best accomplished with a meter that will measure inductance, checking for high impedance "short circuits" amongst the three conductors of the cable. Considerable disassembly may be required to do this properly, (to isolate both ends of the cable) hence the recommendation to call in the service representative.
On our Philips 400T we had a switch on the back of the left console that was marked Low/High, the low settng was used for tungsten filaments and the high setting for LaB6 filaments which required more current to heat the crystal. It may be that this switch was accidently bumped to the high position?
At 4:49 PM -0400 5/13/02, Leland G Hanna wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
-- David R. Hull NASA Glenn Research Center at Lewis Field Advanced Metallics Branch Mail Stop 49-1 21000 Brookpark Road Cleveland, OH 44135
Sergey points out some good facets of file recovery.
What is missing from your post is whether you are using FAT16, FAT32 or NTFS. In a "normal" mode, the OS does not delete the file, but rather, it "marks" it as deleted. This is done by replacing the file name with an initial ? mark. There are variations on this theme. But unless and until the disk is defragmented, the original file is still on the drive. (a good reason to use Norton WipeDisk if you don't want it to remain there) But there are exceptions, of course.
I agree that Norton DiskDoctor is the way to go. This will allow recovery (un-deletion) of files. But beware that if you delete a file and do other disk actions, recovery may be impossible. This is because the prior-used sectors are now marked as available for use. So if you delete a file, then add new files, all or portions of your deleted file's sectors could be used--eliminating any possibility of recovery.
gary g.
At 12:58 PM 5/13/2002, you wrote:
} Hello Jeremy } } Is it possible to recover corrupted JPEG file specifically? Never hear } about that. I could talk about PC/Win platform only. Windows NT itself } (NTFS file system) has internal ability to recover corrupted files } (any). It's called 'checkdisk' I believe. It's in the standard Windows } package. Similar things should be in win2000. You may also run Norton } Disk Doctor on any Win platform - it works great. The things about that: } all these programs are not specific to the JPEG files. So, I am not sure } how it may help in your particular case. By the way, for PC/Win I would } strongly recommend to have Norton Utilities on HD: very useful stuff. Sergey } } At 01:16 PM 5/13/02 +0100, you wrote: } } ------------------------------------------------------------------------ } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
I finally found the software I was looking for. This information was forwarded to me by Michael Nesson, Ph.D. at OSU and a similar message was sent by John Mardinly.
"The company is called Alicona Imaging GmbH. The software product is called MeX. Try www.alicona.com for additional information."
A demo version is available online and the software looks very impressive but the cost is several $K. Thank you for the help.
Dan
**************************************************************************** ****************************************************************** Daniel D. Smolko, Ph.D. Senior Research Scientist & BioChemical Engineer Nanogen, Incorporated 10398 Pacific Center Court San Diego, CA 92121
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Thank you to all who responded to my request for information regarding other software for slide presentation. Some of the suggestions include: (a) http://www.irfanview.com I downloaded this tonight and I find it very easy to use. (b) UPresent from http://www.codeblazer.com/products.html I have not tried this yet (c) Sliderite (d) using HTML (e) JPEGView (f) Other suggestions deal with increasing the computer RAM and data compression.
Our projector has a 1024 x768 resolution and we do paste the full image onto the Powerpoint page and then adjust the size of the image but the problem comes when we try to paste a composite consisting of more than 6 images. Quite often the images appear washed out - the images were captured originally in Tiff format but as I indicated earlier we had to compress the file before pasting.
Thank you all for the information. I will try some of the other suggestions soon.
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
Here here, i recently left clinical area for reseach. the head cyto tech convinced the administrator that he could do the job as good as i could. in six months he trashed the lab 3 diamond knives, and an LKB. an average EM tech. is probly a bad em tech. as for your question. i have seen labs that do 1000/year with just 1.5 techs. i wouldn't want to work in one of those mills. john
Long time lurker, first time poster (well, almost).
We recently upgraded from a video camera to a cooled digital camera that is very sensitive. While doing epifluorescence on our Nikon TE300, we noticed some rather significant variations in the illumination from the mercury lamp, specifically a hot spot filling about 1/4 of the screen. This is not visible through the eyepiece and is not visible with the video camera. I have tried re-aligning the lamp in various ways. This moves the hot spot around but cannot make it go away. I even tried putting a diffuser in the light path. The hot spot is still there. I've had the vendors in, who say we might need a lamp with a bigger arc to fill the field of view.
The following note is posted for a friend who does not have access to the list server;
Joseph M. Oparowski Materials Science Research - Consulting and Failure Analysis Bose Corporation Joseph_Oparowski-at-bose.com The Mountain, M/S 415 Phone: (508) 766-1371 Framingham, MA 01701-9168 Fax: (508) 766-1313
A colleague is looking for someone to install an Amray 3600 FESEM. Please reply directly to
James Greer PVD Products 231 Andover St. Wilmington, MA 01887 (978) 694-9455 jgreer-at-pvdproducts.com
You might be imaging a reflection off of the front of some part of the camera/lens system. Check to make sure that there is no contamination on the forward side of any of the accessible optical elements that could serve as a source of scattered light that would be reflected by another optical element.
John Twilley
Eric Johnston 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 } } Long time lurker, first time poster (well, almost). } } We recently upgraded from a video camera to a cooled digital camera that is } very sensitive. While doing epifluorescence on our Nikon TE300, we noticed } some rather significant variations in the illumination from the mercury } lamp, specifically a hot spot filling about 1/4 of the screen. This is not } visible through the eyepiece and is not visible with the video camera. I } have tried re-aligning the lamp in various ways. This moves the hot spot } around but cannot make it go away. I even tried putting a diffuser in the } light path. The hot spot is still there. I've had the vendors in, who say } we might need a lamp with a bigger arc to fill the field of view. } } Does anybody have any suggestions? } } Eric
Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (giummc-at-rpi.edu) from http://www.msa.microscopy.com/Ask-A-Microscopist.html on Tuesday, May 14, 2002 at 12:37:15 ---------------------------------------------------------------------------
Email: giummc-at-rpi.edu Name: Cindie Giummarra
Organization: Rensselaer Polytechnic Institute
Education: Graduate College
Location: Troy, New York, USA
Question: Hi,
I was wondering which techniques I could use to detect calcium in 15-40ppm amounts in an aluminum alloy?
I am interested in finding out what form the Ca is in and where it is located in the microstructure.
O.k. this is not mciroscopy directly BUT I hope someone out there has an answer.
We're looking for an "adhesive" to glue #3 Whatman filter paper to stainless steel (surface area of ~ 3 sq cm or less) but it must be: (1) sterile or sterilizable, (2) water stable, (3) biologically non-toxic.
Thanks for your suggestions!
Richard E. Edelmann, Ph.D. Electron Microscopy Facility Supervisor 352 Pearson Hall Miami University, Oxford, OH 45056 Ph: 513.529.5712 Fax: 513.529.4243 E-mail: edelmare-at-muohio.edu http://www.emf.muohio.edu
We have an old Nikon Labophot2 and we are in need of a trinoc head. It is currently a dual head scope but we need to convert it so it can handle a digital camera. Currently we have a TriPix RGB (hanging off one of the eyepieces with an adapter) but we're having trouble with dust and spots at 100X oil. I know this is not the optimum configuartion.
Does any one have a suggestion about digital cameras for light microscopes? We are working mostly with H&E (10 -40X) and some blood smears (100X oil). We will be saving images to a website.
Also, I'm looking for anybody who might have a old trinoc head for a Nikon Labophot2 sitting around that might want to sell it.
I'm welcome to all ideas, so send them along.
In the new land of tornadoes,
Paula Sicurello George Washington Univ. Medical Center Dept. of Pathology, Ross Hall rm 505 Electron Microscope Lab 2300 Eye St. Washington, DC 20037 202-994-2930 phone 202-994-2518 fax
Silicone or epoxy compound? Both of them are 'naturally' aseptic- aggressive enough to kill any bacteria unless polymerized.... Silicone when completely polymerized (be sure) is bio-compatible. I mean silicone compound with clear silicone base and strong smell of acetic acid. Sergey
At 11:58 AM 5/14/02, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
_____________________________________
Sergey Ryazantsev Ph. D. Electron Microscopy UCLA School of Medicine Department of Biological Chemistry Box 951737 Los Angeles, CA 90095-1737
I haven't had a chance to test this but I saw a very impressive demonstration by Adobe using their Acrobat program (not the free Acrobat Reader). Creating PDF files and editing them with this software is quite easy and allows almost any program for creation.
Also, properly cured Silicone compounds mostly compatible with hot water, but not with hot steam on repeated exposure, especially pressure seals. Sterilize by boiling, not autoclaving. Try www.nusil.com for more information.
Vitaly Feingold Scientific Instruments and Applications 2773 Heath Lane, Duluth GA 30096 (770)232-7785 ph. (770)232-1791 fax (678)467-0012 mobile
This message is made of 100% recycled electrons. ----- Original Message ----- } From: Sergey Ryazantsev {sryazant-at-ucla.edu} To: {Microscopy-at-sparc5.microscopy.com} Sent: Tuesday, May 14, 2002 6:10 PM
Surprising: silicone rubber (after polymerization of the silicone compound) is extremely stable against the temperature. It widely used in high temperature applications (simplest example: silicone compound for car engines). 121oC which is typical autoclave temperature should not hurt silicone at any instances even with overheated steam... I also check WEB site you suggested and did not find anything about thermal instability of the silicones... Moreover, the curing temperature they suggested is 150oC for 5 hours, which is much longer than autoclave procedure (20-30 min usually). If I remember correctly, people used silicone compound to make molds for the metal... I am sorry, could not agree with you: as I know, silicone is most thermally stable rubber suitable for biological/medical use. Actually, my point was that if you perform procedure at the sterile conditions (laminar cabinet with HEPA filter for instance) you don't have to sterilize the compound. Compound is sterile itself. You DO have to care about sterility of the other parts, but non-polymerized silicone. Sergey
At 08:26 PM 5/14/02, you wrote: } Also, properly cured Silicone compounds mostly compatible with hot water, } but not with hot steam on repeated exposure, especially pressure seals. } Sterilize by boiling, not autoclaving. Try www.nusil.com for more } information. } } Vitaly Feingold } Scientific Instruments and Applications } 2773 Heath Lane, Duluth GA 30096 } (770)232-7785 ph. } (770)232-1791 fax } (678)467-0012 mobile } } This message is made of 100% recycled electrons. } ----- Original Message ----- } From: Sergey Ryazantsev {sryazant-at-ucla.edu} } To: {Microscopy-at-sparc5.microscopy.com} } Sent: Tuesday, May 14, 2002 6:10 PM } Subject: Re: Biosafe adhesive } } } } ------------------------------------------------------------------------ } } 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 } } -----------------------------------------------------------------------. } } } } } } Silicone or epoxy compound? Both of them are 'naturally' aseptic- } } aggressive enough to kill any bacteria unless polymerized.... Silicone } } when completely polymerized (be sure) is bio-compatible. I mean silicone } } compound with clear silicone base and strong smell of acetic acid. Sergey } } } } At 11:58 AM 5/14/02, you wrote: } } } ------------------------------------------------------------------------ } } } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } } } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } } } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } } } -----------------------------------------------------------------------. } } } } } } } } } O.k. this is not mciroscopy directly BUT I hope someone out } there } } } has an } } } answer. } } } } } } We're looking for an "adhesive" to glue #3 Whatman filter paper } to } } } stainless steel (surface area of ~ 3 sq cm or less) but it must be: (1) } } } sterile or } } } sterilizable, (2) water stable, (3) biologically non-toxic. } } } } } } Thanks for your suggestions! } } } } } } } } } } } } Richard E. Edelmann, Ph.D. } } } Electron Microscopy Facility Supervisor } } } 352 Pearson Hall } } } Miami University, Oxford, OH 45056 } } } Ph: 513.529.5712 Fax: 513.529.4243 } } } E-mail: edelmare-at-muohio.edu } } } http://www.emf.muohio.edu } } } } } } "RAM disk is NOT an installation procedure." } } } } _____________________________________ } } } } Sergey Ryazantsev Ph. D. } } Electron Microscopy } } UCLA School of Medicine } } Department of Biological Chemistry } } Box 951737 } } Los Angeles, CA 90095-1737 } } } } Phone: (310) 825-1144 } } FAX (departmental): (310) 206-5272 } } mailto:sryazant-at-ucla.edu } } } } } } } } } }
_____________________________________
Sergey Ryazantsev Ph. D. Electron Microscopy UCLA School of Medicine Department of Biological Chemistry Box 951737 Los Angeles, CA 90095-1737
Dear all, We have a GIF here attached to a JEOL 3010 and something strange has happened to the energy selecting slit. It is far too wide (like a measured width of about 70 eV, when nominally set to 1eV). Is there any user intervention that can fix this problem easily? (e.g. Does anyone understand how to use the Slit Width Calibration function in Filter Control, and would this help?)
Or, is this simply a case for calling the Gatan Service Engineer?
Dear all, Has anybody out there installed a TV Camera for HREM imaging ABOVE the normal viewing screen in a TEM?
We would like to install a TV Camera on a JEOL TEM for focussing HREM images, but there's no space below the Camera due to other attachments being there. Meanwhile, there are a couple of ports free above the viewing screen.
If anyone has any ideas of good cameras / camera manufacturers for this purpose, please contact me.
Previous and present ETEC owners, Does anyone have an ETEC micromanipulator hidden away in a drawer or cabinet? One of my customers has my only complete one and needs a second for a project. Beg, borrow, rent or buy are all options. Thanks.
Ken Converse owner Quality Images third party SEM service 16 Creek Rd. Delta, PA 17314
Morning Eric, Just a guess, but one of the things that is emitted in large quantity is heat (ir?). In the old days when bright light in microscopy always came from a carbon arc, the UV was filtered thru a 1"+ layer of copper sulfate solution to cool off the light (remove the ir?). Now, if I remember, most CCD detectors have a sweet spot in the near or far red (ir?). My guess is that you may be 'seeing' with your CCD what YOU cannot see during visual alignment. I believe that there are barrier filters or N.D. filters in front of the Hg lamp that will accomplish what you want.
Regards,
Fred Monson
Frederick C. Monson, PhD Center for Advanced Scientific Imaging Schmucker II Science Center West Chester University South Church Street and Rosedale West Chester, Pennsylvania, USA, 19383 Phone: 610-738-0437 FAX: 610-738-0437 fmonson-at-wcupa.edu CASI URL: http://darwin.wcupa.edu/casi/ WCUPA URL: http://www.wcupa.edu/ Visitors URL: http://www.wcupa.edu/_visitors/
} ---------- } From: Eric Johnston } Sent: Tuesday, May 14, 2002 8:50 AM } To: Microscopy-at-sparc5.microscopy.com } Subject: Hot spot in epifluorescence } } ------------------------------------------------------------------------ } 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 } } Long time lurker, first time poster (well, almost). } } We recently upgraded from a video camera to a cooled digital camera that } is } very sensitive. While doing epifluorescence on our Nikon TE300, we } noticed } some rather significant variations in the illumination from the mercury } lamp, specifically a hot spot filling about 1/4 of the screen. This is } not } visible through the eyepiece and is not visible with the video camera. I } have tried re-aligning the lamp in various ways. This moves the hot spot } around but cannot make it go away. I even tried putting a diffuser in the } light path. The hot spot is still there. I've had the vendors in, who } say } we might need a lamp with a bigger arc to fill the field of view. } } Does anybody have any suggestions? } } Eric } } }
You may want to try SIMS [Scanning Ion Mass Spectroscopy] [EDX may only be able to do about 1,000 ppm, but that is sample dependent and matrix dependent.]
Peter Tomic Anadigics, Inc.
-----Original Message----- } From: giummc-at-rpi.edu [mailto:giummc-at-rpi.edu] Sent: Tuesday, May 14, 2002 2:20 PM To: Microscopy-at-sparc5.microscopy.com
Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (giummc-at-rpi.edu) from http://www.msa.microscopy.com/Ask-A-Microscopist.html on Tuesday, May 14, 2002 at 12:37:15 ---------------------------------------------------------------------------
Email: giummc-at-rpi.edu Name: Cindie Giummarra
Organization: Rensselaer Polytechnic Institute
Education: Graduate College
Location: Troy, New York, USA
Question: Hi,
I was wondering which techniques I could use to detect calcium in 15-40ppm amounts in an aluminum alloy?
I am interested in finding out what form the Ca is in and where it is located in the microstructure.
We have an EDS detector attached to a 200 kV TEM that is having its crystal changed (to a Si(Li)). The original resolution was 139 eV. Now, depending on the amount of the repair, it could become 138 or 143 eV. My question is : is 143 eV worse than 138 eV in practise ? Does one notice the difference ?
I appreciate any ideas.
Isabel
Isabel Nogueira Lab Technicien Instituto Superior Técnico Materials Department Avenida Rovisco Pais 1049-001 Lisboa Portugal tel.: +351 218418123 fax: +351 218418120 email: isabeln-at-popsrv.ist.utl.pt
I suppose the issue depends on how you use your detector and which elements you examine. If it is for elements up through arsenic, you should have little trouble with overlaps and 143 eV resolution ought to be fine. If you are looking at heavier metals with lots of overlaps, you may want to hold out for the better resolution. For example, last week I was looking at a Pb-Bi-Sn-Cd fusible alloy. That made for plenty of overlaps. Even so, I think my results were good even without operating in the highest resolution mode.
Our EDS offers 20, 10, and 5 eV/channel modes. Thus you are only talking about a difference of 1/4th of a channel in the 20 eV/channel mode which we use most of the time. I don't think you would notice it. But that is only my guess.
Warren
At 02:39 PM 5/15/02 +0100, you wrote:
} Dear colleagues, } } We have an EDS detector attached to a 200 kV TEM that is having its crystal } changed (to a Si(Li)). } The original resolution was 139 eV. Now, depending on the amount of the } repair, it could become 138 or 143 eV. } My question is : is 143 eV worse than 138 eV in practise ? Does one notice } the difference ? } } I appreciate any ideas. } } Isabel } } Isabel Nogueira } Lab Technicien } Instituto Superior Técnico } Materials Department } Avenida Rovisco Pais } 1049-001 Lisboa } Portugal
------------------------------------------- No files should be attached to this message ------------------------------------------- Warren E. Straszheim, Ph.D. Materials Analysis and Research Lab Iowa State University 23 Town Engineering Ames IA, 50011-3232
} O.k. this is not mciroscopy directly BUT I hope someone out there } has an } answer. We're looking for an "adhesive" to glue #3 Whatman filter paper to } stainless steel (surface area of ~ 3 sq cm or less) but it must be: (1) } sterile or sterilizable, (2) water stable, (3) biologically non-toxic. } } Richard -
My son-in-law makes and repairs diamond scalpels (he started with diamond EM knives, but decided that surgeons are less fussy & more clumsy than microscopists). He, and the other manufacturers, cements the blades into steel or titanium handles with a 2-part epoxy glue that can take autoclave temperatures.
Caroline
Caroline Schooley Project MICRO Coordinator Microscopy Society of America Box 117, 45301 Caspar Point Road Caspar, CA 95420 Phone/FAX (707)964-9460 Project MICRO: http://www.msa.microscopy.com/ProjectMicro/PMHomePage.html Intertidal invertebrates: http://www.fortbragg.k12.ca.us/AG/marinelab.html
I have recently been thinking of purchasing the Nikpn Coolpix 995 for digital photgraphy but I read some of the thread from last year regarding attaching this camera to a microscope. I have attached it and for what I was doing at the time it was suitable. Can anyone suggest other digital cameras in the same price range that will do microscopy work (compound and dissecting)(macro and micro), good outside and indoor photos and can be used to photograph electrophoresis gels. Thanks Debbie
As stated previously, your average tech would not be a good thing. I have been in a clinical lab for the past 18 years. When I first came to this lab it had 3 techs, myself included with no less then 8 years EM experience each. We were processing around 1850 specimens per year with a turn around time of less than 48 hours (the specimens had been in glut for at least overnight). About half of these were cut and viewed for diagnosis. This is an average of 7 processed per day and 4 per day being cut and viewed. Some days were more some less. I remember at least one day where we processed 15 specimens. So as you can see, the question you should ask is not how many specimens can be processed, but how many can be cut and scoped successfully in a day. Anyone that can follow a protocol can process but only an experienced tech can successfully cut, stain, scope, and print a specimen. If s/he is the only tech in the lab, then IMHO the most one could expect would be maybe 4 or 5 specimens per day if s/he were doing everything (the processing, cutting etc) and this would be pushing the limit to do everyday day in and day out. If the specimens were in blocks, then one may be able to do 8 or more in a day depending on the number of pictures taken and the speed of the print processor in the darkroom, again not something I would want to do every day. If your images are acquired digitally, then that would need to be accounted for in the scheme of things.
Mannie Steglich Tech Dir E M Lab U T M D Anderson Cancer Center
I'm trying to help a colleague refine their technique for a 3D reconstruction project. They work with kidney. They are trying to reconstruct all of the thin loops of Henle (approx 15um in diameter) through a depth of about 3-4 mm. In a nutshell, their current protocol is:
* formaldehyde fix & process kidney tissue for TEM (w/o OsO4) * embed in Spurrs (normal hardness) * cut 1um sections with a glass knife, sampling every 5um * etch the epoxy from the sections and perform immunohistochemistry * capture images of the sections and software align them for 3D reconstruction
Their biggest complaint is aligning the sections. My thought was that this might be as a result of compression due to sectioning (the block faces are pretty large). Occasional wrinkles in the plastic don't help matters.
As we talked about the problem there were a couple of issues that I raised. I'd appreciate feedback from the list, since I've not done any 3D work before.
* would a harder formulation of Spurrs be a better choice? * would a different epoxy altogether be a better choice? * if a different epoxy, how about something like LRGold (apologies to vendors of competing products), a methacrylate-type plastic that could be embedded at a lower temp and might be better overall for their immuno-reactions (but might be more prone to shrinkage and/or compression artifacts)?
Yours, Doug Cromey
.................................................................... : Douglas W. Cromey, M.S. Dept. of Cell Biology & Anatomy : : Research Specialist, Principal University of Arizona : : (office: AHSC 4212A) P.O. Box 245044 : : (voice: 520-626-2824) Tucson, AZ 85724-5044 USA : : (FAX: 520-626-2097) (email: Cromey-at-Arizona.edu) : :...................................................................: http://swehsc.pharmacy.arizona.edu/exppath/ Home of: "Microscopy and Imaging Resources on the WWW"
The majority suggest that there is some kind of reflection on one or more of the lens surfaces that's causing the hot spot, especially from the camera adapter (in my case, the adapter has no lens so that's out).
The other suggestion was that the hot spot is due to IR, which CCDs can be especially sensitive to. I need to find out if there is an IR blocker in light path or on the camera itself.
Thanks for all the helpful suggestions. I'll keep you updated.
} I have a relatively old Wild dissecting scope that needs } repair/service. Does anyone know a good place to have that done in the } Bay area, preferably near Stanford? Is this the kind of thing that } Universities typically have standing contracts with someone for?
Maybe more important than the quoted detector resolution is how you choose to run the EDS system. Using small amplifier time constants and high counting high rates can degrade the actual resolution a lot more than just a few eV.
For historic reasons, EDS detector resolution is quoted at the energy of Mn K-alpha x-rays (5.4 keV). However, the EDS resolution is actually has energy dependent and energy independent contributions, so the x-ray peaks at O-K, for example will be much narrower than those at Mn or Fe-K. Degrading the detector resolution by adding (energy independent) electronic noise will broaden the low-energy peaks much more than it does the high-energy ones.
Warren's comment about heavy elements and peak overlaps might need clarification. For EDS of heavy elements in a TEM (as opposed to an SEM), you can use the K or L-shell x rays with energies up to 20, 40 keV, or even higher energies to avoid significant overlaps. The problem with peak overlaps arises when you want to include light elements in the analyses and the K-peaks from those elements overlap with higher-shell x-rays (e.g., L or M) from the heavy elements in your sample. In that case, you might want better resolution.
Larry
---------- From: Warren E Straszheim Sent: Wednesday, May 15, 2002 7:11 AM To: Microscopy-at-sparc5.microscopy.com Subject: Re: EDS detector resolution
------------------------------------------------------------------------ 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 suppose the issue depends on how you use your detector and which elements you examine. If it is for elements up through arsenic, you should have little trouble with overlaps and 143 eV resolution ought to be fine. If you are looking at heavier metals with lots of overlaps, you may want to hold out for the better resolution. For example, last week I was looking at a Pb-Bi-Sn-Cd fusible alloy. That made for plenty of overlaps. Even so, I think my results were good even without operating in the highest resolution mode.
Our EDS offers 20, 10, and 5 eV/channel modes. Thus you are only talking about a difference of 1/4th of a channel in the 20 eV/channel mode which we use most of the time. I don't think you would notice it. But that is only my guess.
Warren
At 02:39 PM 5/15/02 +0100, you wrote:
} Dear colleagues, } } We have an EDS detector attached to a 200 kV TEM that is having its crystal } changed (to a Si(Li)). } The original resolution was 139 eV. Now, depending on the amount of the } repair, it could become 138 or 143 eV. } My question is : is 143 eV worse than 138 eV in practise ? Does one notice } the difference ? } } I appreciate any ideas. } } Isabel } } Isabel Nogueira } Lab Technicien } Instituto Superior Técnico } Materials Department } Avenida Rovisco Pais } 1049-001 Lisboa } Portugal
------------------------------------------- No files should be attached to this message ------------------------------------------- Warren E. Straszheim, Ph.D. Materials Analysis and Research Lab Iowa State University 23 Town Engineering Ames IA, 50011-3232
------------------------------------------------------------------------ The Microscopy ListServer -- Sponsor: The Microscopy Society of America
} O.k. this is not mciroscopy directly BUT I hope someone out there } has an } answer. We're looking for an "adhesive" to glue #3 Whatman filter paper to } stainless steel (surface area of ~ 3 sq cm or less) but it must be: (1) } sterile or sterilizable, (2) water stable, (3) biologically non-toxic. } } Richard -
My son-in-law makes and repairs diamond scalpels (he started with diamond EM knives, but decided that surgeons are less fussy & more clumsy than microscopists). He, and the other manufacturers, cements the blades into steel or titanium handles with a 2-part epoxy glue that can take autoclave temperatures.
Caroline
Caroline Schooley Project MICRO Coordinator Microscopy Society of America Box 117, 45301 Caspar Point Road Caspar, CA 95420 Phone/FAX (707)964-9460 Project MICRO: http://www.msa.microscopy.com/ProjectMicro/PMHomePage.html Intertidal invertebrates: http://www.fortbragg.k12.ca.us/AG/marinelab.html
Hello, Our glow discharge unit is becoming unreliable, and we are thinking about replacing it. We have contemplated having a dedicated stand alone unit versus going with a large vacuum evaporator multi-function system. I send this message out so that vendors can respond directly to me, and also as a solicitation for what technology has/hasn't worked for others. Thanks in advance, Randy Nessler University of Iowa Central Microscopy Research Facility Iowa City, Iowa 52358 Phone 319-335-8142 Fax 319-384-4469
Just another posting about digital microscope adaptors. I am looking for informatio leading to the ordering and purchase of an adaptor for the Olympus E20N digital camera.
At the college lab where I will be teaching as an adjunct this summer, a new toy has been purchased: an Olympus E20N digital camera. Some discussion has focused on purchase of a microscope attachment. The attachment that has been recommended by one of the staff attaches to the 62mm filter ring threads of the camera. I have two scopes that I use in teaching, each of them w/ c. 45. eyetube inclination angles; there is no trinocular tube available. I fear the forces of attaching a camera to a scope by the filter ring at such an angle would be unhealthy for the camera. The camera is a hefty one.
Alan Davis
-- Alan E. Davis Science Department Marianas High School PMB 30, Box 10006, Saipan, MP 96950 Northern Mariana Islands adavis-at-saipan.com
"An inviscid theory of flow renders the screw useless, but the need for one non-existent." ---Lord Raleigh(aka John William Strutt),or else his son, Jr., who was also a scientist.
Dear Debbie, I recently saw a new Sony camera with a large lens that can focus down to about one inch and claims to have better low-light performance than most digitals. It is a 5 megapixel and sells for about what the Nikon 995 did when it was first introduced (~$1650.00CAN). I'm sorry, I don't know the model number, but it is hard to miss, since it looks funny with a tiny digital camera body attached to a large, complex optical lens. It might best suit your multiple needs. At 10:35 AM 5/15/02 -0400, you wrote:
} I have recently been thinking of purchasing the Nikpn Coolpix 995 for } digital photgraphy but I read some of the thread from last year } regarding attaching this camera to a microscope. I have attached it and } for what I was doing at the time it was suitable. Can anyone suggest } other digital cameras in the same price range that will do microscopy } work (compound and dissecting)(macro and micro), good outside and indoor } photos and can be used to photograph electrophoresis gels. Thanks } Debbie } Regards, Mary
Mary Mager Electron Microscopist Metals and Materials Engineering University of British Columbia 6350 Stores Road Vancouver, B.C. V6T 1Z4 CANADA tel: 604-822-5648 e-mail: mager-at-interchange.ubc.ca
Arizona State University Center for Solid State Science is seeking qualified candidates to fill the position Engineer Senior or Principal. Level and salary will be determined based on qualifications. This is a full time, benefit eligible position. This position is responsible for maintaining high levels of performance in analytical high-resolution electron microscopes particularly electrical, magnetic and mechanical stability, while concurrently developing these systems to achieve higher levels of performance, including computer interfacing.
Complete qualifications and application information please refer to SR 108236 at www.asu.edu/hr/jobs/. Application deadline is May 28, 2002 and every two weeks thereafter until search is closed.
John C. Wheatley Lab Manager Arizona State University Center for Solid State Science PSA-213 BOX 871704 Tempe, AZ 85287-1704
I am not at my office at the moment (using webmail) so I cannot check directly but I have some filters from way back which I think I bought from Schott (I have no connection with the company!).
Try going to
www.google.com
and searching on
optical glass filters
or something similar. Schott comes up as do many others of course.
Good luck
Gareth
Gareth Morgan MPhil MSc FIBMS, Institute for Microbiology, Pathology and Immunology (IMPI), H5, Karolinska Institutet, Lindhagensgatan 92, Box 12773, S 112 96, Stockholm Sweden
----- Original Message ----- } From: Sergey Ryazantsev {sryazant-at-ucla.edu} To: {Microscopy-at-sparc5.microscopy.com} Sent: Wednesday, May 15, 2002 2:23 AM
I have seen today Panasonic Lumix DMC-LC5A with Leica lenses and looks also very good. 3,9 Mega pixels just for AUS dollars 1775 Ricardo Keep care and be of good cheer
Regards
(name) Vratislav Richard Eugene Maria John Baptist (surname) of Bejsak (Bayshark)-Colloredo-Mansfeld (title) 84 duke of Siebenlügner
websites: http://www.coleoptera.org. and http://www.egroups.com/group/coleoptera
University of Sydney The Wentworth Bldg., B 62 NSW 2006 AUSTRALIA phone : +61 414 540 465 email: vratislav-at-bigfoot.com ICQ: 13610107
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).
http://www.mir.com.my/rb/photography/hardwares/classics/olympusom1n2/om1/om1 manual/index5.htm [an old Olympus OM1 site with a 'massive' camera stand to isolate it from scope]
http://www.lensadapter.com/optical_article.htm [here's a guy who has your problem] http://www.lensadapter.com/default.htm [looks like just what you need!!!!]
These last two were the best finds of the exercise. Hope it helps.
Fred
} ---------- } From: Alan E. Davis } Sent: Wednesday, May 15, 2002 6:26 PM } To: microscopy-at-sparc5.microscopy.com } Subject: More digiterata: Microscope attachment for Olympus E20N? } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Just another posting about digital microscope adaptors. I am looking for } informatio leading to the ordering and purchase of an adaptor for the } Olympus E20N digital camera. } } At the college lab where I will be teaching as an adjunct this summer, a } new toy has been purchased: an Olympus E20N digital camera. Some } discussion has focused on purchase of a microscope attachment. The } attachment that has been recommended by one of the staff attaches to the } 62mm filter ring threads of the camera. I have two scopes that I use in } teaching, each of them w/ c. 45. eyetube inclination angles; there is no } trinocular tube available. I fear the forces of attaching a camera to a } scope by the filter ring at such an angle would be unhealthy for the } camera. The camera is a hefty one. } } Alan Davis } } -- } Alan E. Davis } Science Department } Marianas High School } PMB 30, Box 10006, } Saipan, MP 96950 } Northern Mariana Islands } adavis-at-saipan.com } } } "An inviscid theory of flow renders the screw useless, but the need } for one non-existent." } ---Lord Raleigh(aka John William Strutt),or else } his son, Jr., who was also a scientist. } }
The Army Research Laboratory, Adelphi MD (http://www.arl.army.mil) is about to advertise a position for an experienced Ph.D. level TEM specialist. We are looking for someone with experience and publications in the TEM of semiconductor materials/devices. Experience with or interest in Auger electron spectroscopy, MOCVD, wide bandgap materials, and FIB sample preparation would be beneficial. We have a JEOL 2010 and a JEOL 2010F with EDX. Applicants MUST BE US CITIZENS. ARL is an equal opportunity employer. Please e-mail resumes directly to me, although, this will not constitute an official application for the position which must be done by responding to the official posting.
Sincerely, Matthew Ervin, Ph.D. MErvin-at-ARL.Army.mil
M/S: AMSRL-SE-RL US Army Research Laboratory 2800 Powder Mill Road Adelphi, MD 20783-1197
Disclaimer: The opinions and views expressed above are those of the author and do not necessarily represent those of the U.S. Army Research Laboratory or any other government agency
The camera you refer to is the Sony DSC-F707. It has 5MP resolution, a Zeiss zoom lens, USB interface and uses Memory Stick media for storage. http://www.sonystyle.com/digitalimaging/P_Feature_F707.shtml
} I recently saw a new Sony camera with a large lens that can focus } down to about one inch and claims to have better low-light } performance than most digitals.... ... it is hard to miss, since } it looks funny with a tiny digital camera body attached to a } large, complex optical lens.
The Nikon Coolpix 5000 is also a 5MP camera with a Nikon zoom lens, .75 inch minimum focus, and accepts compact flash media. It will also shoot 320x240 Quicktime movies(the Sony also has a "video" mode). Image quality is excellent. In addition to standard exposure controls, the CP5000 also has adjustments for contrast, noise reduction, sharpening and saturation. An electronic release is also available to reduce potential vibration from depressing the shutter or to do interval timing. Microscope couplers are readily available for the 5000 to fit most microscopes. http://www.nikonusa.com/usa_product/product.jsp?cat=1&grp=2&productNr=25501 or we have a PDF available.
} Can anyone suggest other digital cameras in the same price range } that will do microscopy work (compound and dissecting)(macro and } micro), good outside and indoor photos and can be used to photograph electrophoresis gels.
George
George Laing National Graphic Supply ph 800.223.7130 x3109 f 800.832.2205 email scisales-at-ngscorp.com
Hello all, would anybody have any thoughts on the Retiga 1300 Monochromatic cooled CCD camera (for fluorescent microscopy) a and its price: CAN$ 12,300.00 (CAN$ = US$ 0.63).
Thank you for your help, Sincerely,
Sarka Lhotak
Hamilton Regional Cancer Centre McMaster University Hamilton, Ontario, Canada
Hi All, We have a EMITech K850 Critical Point Dryer and a new tank of Research Grade CO2, and we have problems. The runs have all of a sudden become VERY inconsistent.
Ambient temp in the Lab is around 18oC After cooling the chamber to 5oC and opening the Inlet valve, the pressure rises to 750psi at which is will remain for at least an hour with all valves closed. With the Inlet valve open, however, and waiting for liquid CO2 to show in the sight glass, the temperature begins to rise and does so to around 10oC at which point the fluid begins to rise in the glass to about 1/8 of the 1cm diameter. If I re-cool the chamber to 5oC, the fluid disappears. If I wait for up to 3 minutes, one of two things happens. 1. the fluid reappears and rises to 1/2 the sight window, or 2. I see nothing until I release the pressure and for a brief period note the fluid level show at the very top of the sight glass and fall and disappear very rapidly. After the first run, which I cannot control, I cannot merely recyle the unit. I have to wait an hour to demonstrate another unsatisfactory test.
If anyone can help me ferret out this poltergeist, I would be most appreciative. I must say that I am convinced that I am dealing with a daemon from the PChem lab.
I attached my Polaron CPD, which is much simpler in design and saw the same initial 750 psi but NO fluid accumulation after watching for 10min.
Hoping that it is NOT that terrible tank with the broken siphon (again after all these years),
Fred Monson
Frederick C. Monson, PhD Center for Advanced Scientific Imaging Schmucker II Science Center West Chester University South Church Street and Rosedale West Chester, Pennsylvania, USA, 19383 Phone: 610-738-0437 FAX: 610-738-0437 fmonson-at-wcupa.edu CASI URL: http://darwin.wcupa.edu/casi/ WCUPA URL: http://www.wcupa.edu/ Visitors URL: http://www.wcupa.edu/_visitors/
It's a nice description of a home made adaptor to fit a Nikon CoolPix on a microscope, using the tripod thread insted of the filter ring threads of the camera. I don't know if the Olympus E20N has such a thread, but it gives some idee how to build something which works well and is not expensive.
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
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } Just another posting about digital microscope adaptors. I am looking } for informatio leading to the ordering and purchase of an adaptor for } the Olympus E20N digital camera. } } At the college lab where I will be teaching as an adjunct this summer, } a new toy has been purchased: an Olympus E20N digital camera. Some } discussion has focused on purchase of a microscope attachment. The } attachment that has been recommended by one of the staff attaches to } the 62mm filter ring threads of the camera. I have two scopes that I } use in teaching, each of them w/ c. 45. eyetube inclination angles; } there is no trinocular tube available. I fear the forces of attaching } a camera to a scope by the filter ring at such an angle would be } unhealthy for the camera. The camera is a hefty one. } } Alan Davis } } -- } Alan E. Davis } Science Department } Marianas High School } PMB 30, Box 10006, } Saipan, MP 96950 } Northern Mariana Islands } adavis-at-saipan.com } } } "An inviscid theory of flow renders the screw useless, but the need } for one non-existent." } ---Lord Raleigh(aka John William Strutt),or else } his son, Jr., who was also a scientist. }
I don't think you will see the difference between 143 and 138 resolution there are many factors that come into play as previously mentioned. Another one is are you replacing the window on your detector also. There are an assortment of different windows that have different energy line curves and strengths. Some may be more suited to your application that is if you are doing something so touchy that 138 resolution to 143 resolution is going to come into play. Why did you need to replace your crystal? Are you replacing your F. E. T. also, as that will effect the detector resolution as well.
Sorry for intruding with a non-microscopy question, but I am looking for feedback on a nationwide ISP. My present ISP has dropped their East Coast dial-ups, and I need access when I travel.
I am looking for the least-intrusive (i.e. not AOL) nationwide ISP. Any suggestions?
Please reply privately unless you have some information you would like the entire list to see.
For those who order CO2-w/siphon tube for critical point drying.
Do you order:
the 'Research Grade' CO2 (-at-$300) or
the standard grade CO2 (-at-$7)?
Thanks,
Fred Monson
Frederick C. Monson, PhD Center for Advanced Scientific Imaging Schmucker II Science Center West Chester University South Church Street and Rosedale West Chester, Pennsylvania, USA, 19383 Phone: 610-738-0437 FAX: 610-738-0437 fmonson-at-wcupa.edu CASI URL: http://darwin.wcupa.edu/casi/ WCUPA URL: http://www.wcupa.edu/ Visitors URL: http://www.wcupa.edu/_visitors/
The Sony F707, Nikon 5000, Olympus E20N and Minolta Dimage 7 all use the same 5 Mega Pixel Sony CCD. Reviews, and test photos comparing resolution, color response and S/N characteristics can be found at this web site: http://www.dpreview.com/ The way I read it, the Sony F707 beats them all quite handily. In addition, the lens is internal focusing, so the end of the camera doesn't move during focusing or poweron/poweroff. In addition, the body with the display on it tilts so that it can be viewed conveniently while mounted vertically. This would be a good to adapt to a microscope, but I do not know if anyone has built a commercially available adapter.
John Mardinly
-----Original Message----- } From: George Laing [mailto:scisales-at-ngscorp.com] Sent: Thursday, May 16, 2002 11:18 AM To: MSA Microscopy Society of America
The camera you refer to is the Sony DSC-F707. It has 5MP resolution, a Zeiss zoom lens, USB interface and uses Memory Stick media for storage. http://www.sonystyle.com/digitalimaging/P_Feature_F707.shtml
} I recently saw a new Sony camera with a large lens that can focus } down to about one inch and claims to have better low-light } performance than most digitals.... ... it is hard to miss, since } it looks funny with a tiny digital camera body attached to a } large, complex optical lens.
The Nikon Coolpix 5000 is also a 5MP camera with a Nikon zoom lens, .75 inch minimum focus, and accepts compact flash media. It will also shoot 320x240 Quicktime movies(the Sony also has a "video" mode). Image quality is excellent. In addition to standard exposure controls, the CP5000 also has adjustments for contrast, noise reduction, sharpening and saturation. An electronic release is also available to reduce potential vibration from depressing the shutter or to do interval timing. Microscope couplers are readily available for the 5000 to fit most microscopes. http://www.nikonusa.com/usa_product/product.jsp?cat=1&grp=2&productNr=25501 or we have a PDF available.
} Can anyone suggest other digital cameras in the same price range } that will do microscopy work (compound and dissecting)(macro and } micro), good outside and indoor photos and can be used to photograph electrophoresis gels.
George
George Laing National Graphic Supply ph 800.223.7130 x3109 f 800.832.2205 email scisales-at-ngscorp.com
I am trying to interface a PC to an Oxford eXL/Lemas system on a JEOL 6300 SEM in order to get external control of the stage. Has anyone tried this and/or do you have any suggestions for getting this to work?
Connections:
(1) eXL (main Oxford control computer using Genie OS) {-{6 pin "LaserBus" & 15 pin stage sync.}-} Lemas (stage motherboard and motor drivers)
(2) Lemas {-{15 pin cable}-} joystick & keypad
(3) Lemas {-} stepper motors & limit
Thanks! ************************************************************************* Frank E. Jones email: jonesfe-at-darkwing.uoregon.edu Department of Physics URL: http://darkwing.uoregon.edu/~jonesfe Office: 189b Klamath Lonergan Lab (Chemistry) University of Oregon Office Phone: (541)346-0977 -------------------------------------------------------------------------
The I.R., in my opinion, seems the likely suspect for the hotspot. I took an optical microscope and deliberately converted it into an IR.. reflected light microscope to image through crystalline compounds like GaAs. What I did was put a filter in the path that blocked the visible light but was a bandpass to I.R. The I.R. naturally is generated by the illuminator. Of course the human eye cannot see into the infra-red but a CCD camera can and does and that is used for imaging and recording vis-a-vis a monitor. I removed the I.R. blocking filter from a B/W camera [just in front of the CCD array to make this work] I also have what you described as a "hot spot." I am trying to diffuse this with a filter that will still transmit I.R. In your case you may need an I.R. blocking filter as you stated. I am looking at Edmund Scientific for a low budget solution.
Please let us know if, or when, you find a solution.
Regards,
Peter Tomic Anadigics, Inc.
-----Original Message----- } From: Eric Johnston [mailto:ericdj-at-seas.upenn.edu] Sent: Wednesday, May 15, 2002 11:09 AM To: Microscopy-at-sparc5.microscopy.com
Hi all
wow, I got a lot of really useful replies.
The majority suggest that there is some kind of reflection on one or more of the lens surfaces that's causing the hot spot, especially from the camera adapter (in my case, the adapter has no lens so that's out).
The other suggestion was that the hot spot is due to IR, which CCDs can be especially sensitive to. I need to find out if there is an IR blocker in light path or on the camera itself.
Thanks for all the helpful suggestions. I'll keep you updated.
I have a dual gun Gatan ion thinner that runs a 1500W oil diffusion pump.
The rules at Brooklyn College require no heat down the drain and water conservation. Thus I need a recirculating chiller. Current lab chillers are $4,000 and up however the pump doesn't require constant temperature so I don't see why an expensive controller, etc is necessary.
Any ideas for a recirculating chiller that is less expensive?
Also any US government labs with a surplus recirculator. It can be donated to an American University.
Thanks, Gordon Nord Environmental Science Institute Brooklyn College, Brooklyn, NY gnord-at-mindspring.com
I hope you don't mind my intrusion onto your list sever. It was suggested by the business office that I post my question here.
I am an amateur microscopist that has dabbling on and off since grade school, exploring the world of the miniature, and interesting views of the ordinary.
I have recently become more serious about this "hobby", and have adapted a digital camera to the photo tube of an optical microscope.
I am hoping to find some type of amateur microscopy association(s) that would help enhance my work and enjoyment. My web search only turned up a group in the UK, and I was hoping to find something "closer to home" (Wisconsin, USA).
Thank you kindly;
John W. Raffensperger, Jr. IS Manager Helwig Carbon Products, Inc.
Gordon, I prefer the Neslab CFT 25 chiller, either digital or analog. The work just fine for a small DP and are very reliable. Check out LABx or a reseller like Bid Service. They usually have some in stock, around $1K.
Gary M. Easton Scanners Corporation Third Party SEM Service
No financial interest in any of the above companies(except mine of course).
----- Original Message ----- } From: "Gordon Nord" {gnord-at-mindspring.com} To: {Microscopy-at-sparc5.microscopy.com} Sent: Saturday, May 18, 2002 11:26 AM
Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (kchamusco-at-mail.ifas.ufl.edu) from http://www.msa.microscopy.com/Ask-A-Microscopist.html on Saturday, May 18, 2002 at 16:01:58 ---------------------------------------------------------------------------
Question: I'm sorry if I should be usinf the list serve but this is the only page I could find to ask a question. I have been working with corn pollen and trying to embed it in LR White resin for immunolabeling in TEM. I thought I had this problem solved, but, apparently I don't. When I get my pollen through the EtOH series up to 95% it looks very good, but when I try to embed it in the resin it collapses. I have tried putting it in resin/EtOH at 20% steps and directly embedding it in 100% resin. The 20% stepwise series seems to be the least destructive and I can get partially collapsed pollen sometimes. I really need to be able to see inside a "fluffy" whole, uncollapsed pollen grain. Is there anyone who can help with this before I pull out the rest of my hair? If necessary to know, I fix in 4% paraformaldehyde + 0.5% gluteraldehyde + 4% sucrose + 0.3% tween {to get the samples to sink}. I vacuum infiltrate for 5 minutes then I leave them in the fridge overnight. I then rinse with PBS and send through a 10% EtOH series{anything greater causes the pollen to collapse}. Then the rest is as I described above. Thanks, Karen
If you use a CCD or CMOS camera you need an IR filter some where. Most color cameras have some filtering but not all. Many monochrome cameras do not have any filtering.
IR light will be out of focus as well as causing hot spots. Silicone in a CCD camera is sensitive into IR light to 1000 nm. With the sensitivity at 800 nm being high enough to cause some problems. A curve with and with out IR blocking filters are given here: http://www.edmundoptics.com/techsupport/DisplayArticle.cfm?articleid=266
Gordon
Gordon Couger Stillwater, OK www.couger.com/gcouger } From: "Peter Tomic" {PTomic-at-anadigics.com} : Eric & Co.; : : The I.R., in my opinion, seems the likely suspect for the hotspot. I took : an optical microscope and deliberately converted it into an IR.. reflected : light microscope to image through crystalline compounds like GaAs. What I : did was put a filter in the path that blocked the visible light but was a : bandpass to I.R. The I.R. naturally is generated by the illuminator. Of : course the human eye cannot see into the infra-red but a CCD camera can and : does and that is used for imaging and recording vis-a-vis a monitor. I : removed the I.R. blocking filter from a B/W camera [just in front of the CCD : array to make this work] I also have what you described as a "hot spot." I : am trying to diffuse this with a filter that will still transmit I.R. In : your case you may need an I.R. blocking filter as you stated. I am looking : at Edmund Scientific for a low budget solution. : : Please let us know if, or when, you find a solution. : : Regards, : : Peter Tomic : Anadigics, Inc. : : : : } From: Eric Johnston [mailto:ericdj-at-seas.upenn.edu] : : : wow, I got a lot of really useful replies. : : The majority suggest that there is some kind of reflection on one or more : of the lens surfaces that's causing the hot spot, especially from the : camera adapter (in my case, the adapter has no lens so that's out). : : The other suggestion was that the hot spot is due to IR, which CCDs can be : especially sensitive to. I need to find out if there is an IR blocker in : light path or on the camera itself. : : Thanks for all the helpful suggestions. I'll keep you updated. : : Eric : :
In about 6 months time I will have to move my microscopes into a newly re-furbished two-storey building. The chillers for the FEI CM120 and Hitachi 4700 may have to be located on the roof, at about 8.5 metres from ground level. I would like to hear from anyone who has considered this, and would particularly value the first-hand experiences of anyone who has already tried it. Are the pumps in standard chillers capable of dealing with an 8-metre head?
We had a Nesslab unit with a pump in our 4th floor fan loft. Our CM12 and SEM were located on the first floor.
I installed pressure gauges at the inlet and outlet lines where they enter the labs. Typical readings on the first floor were 55 PSI on the inlet (from Nesslab) and 15 PSI on the return outlet after going through our scopes. This 15 psi 'back pressure' was simply the pressure of the water standing in the pipe that was 3-4 floors or about 30-35 feet high. The first floor inlet pressure was then 40 PSI + 15 PSI or 55 PSI to the scopes. This is only a net pressure difference of 40 PSI across your scopes.
Upstairs on the outlet side of the Neslab, the pressure gauge at the unit in the fan loft was 40 psi. The 'suction' or inlet at the Nesslab read zero. The buffer tank is open to air. YOUR chiller will not even notice any pressure difference but you will get a loss of 15 PSI to your instruments as shown above.
The net effect was that we had an extra 15 PSI on the whole system on the first floor even when the pump was turned OFF. Don't remove any lines on instruments without shutting both the return and the supply lines OFF.
This pressure worked out to 5 PSI per floor for the three floors above us. I think you will see about 15 PSI back pressure on your instruments on the first floor.
We were forced to install a system that runs off our HVAC chilled water through two heat exchangers in series. It has automatic city water chilling for backup. The temperature of city water is not constant throughout the year. The last heat exchanger and pump is on the first floor and eliminates the back pressure problem. You might consider a heat exchanger and pump on your floor to eliminate the back preesure. My CM 12 can handle much higher pressures. Your does too I believe.
As for your problems: Run DI or distilled water on a CM series scope. Never use chloramine-T because of chloride pit corrosion of SS fittings. Check with Philips service.
Make sure you have a DI water pump to keep the recirc' cooling tank topped off. If you have a leak on the first floor, then you will empty any open buffer tank 'upstairs' fast.
We had a small pump tied into a big DI water tank to deliver enough water to buy us some time to react to a leak problem. It automatically topped off the buffer tank. Also if I drained any water out on the first floor to change the water, it pumped in the required replacement amount without going upstairs.
You need someone in the group to go around and check that all plastic connections are water tight and secure to avoid draining the buffer tank over a weekend, say. Use brass tubing inserts and hose clamps. Make sure all plastic solvent welds are secure.
Use good rubber pressure hose where possible.
You might need a remote temperature light and readout in the first floor hallway to tell someone when there is a problem. This wasn't that effective an alarm system for us. People just walked by without noticing a problem. SO.......
I also have in my lab a small cheap audible temp alarm that has the probe fitted under the chilled water insulation. It is set to go off if any minute temperature rise occurs. I bought this from McMaster-Carr Hardware supply. If it even chirps, I go check the system light and temp readout down the hall, check all pressure readings, and go up to the fan loft and watch the freon compressor cycle. This alarm can also alert you to a partial loss in freon before a sudden total system failure and it allows one to shut down all instruments safely and to notify maintainence of a slight loss in cooling. I highly recommend this alarm.
We originally installed L-type copper 1 inch manifold lines from the fan loft to the first floor and the labs. We tore all that out and now use CPVC dark gray plastic pipe, I believe. This was done to avoid green copper carbonate build up in the RETURN--RETURN lines after diffusion pumps.
Hope this helps.
Paul Beauregard Senior Research Associate
} } In about 6 months time I will have to move my microscopes into a newly } re-furbished two-storey building. The chillers for the FEI CM120 and } Hitachi 4700 may have to be located on the roof, at about 8.5 metres } from ground level. I would like to hear from anyone who has } considered this, and would particularly value the first-hand } experiences of anyone who has already tried it. Are the pumps in } standard chillers capable of dealing with an 8-metre head? } } Chris } } } }
Morning All, For those who are interested in the responses to my last question, here's the dope.
I received 9 responses from VERY reputable sources. NONE used what I called 'Research Grade' CO2 NONE paid more than ~$40, and most paid {$20 / tank Most ordered what they called "bone dry" CO2 One used a hot water pipe heating strip for 1hr before use to insure access to entire liquid charge in tank.
Appreciation to all for your help and advice.
Fred Monson
Frederick C. Monson, PhD Center for Advanced Scientific Imaging Schmucker II Science Center West Chester University South Church Street and Rosedale West Chester, Pennsylvania, USA, 19383 Phone: 610-738-0437 FAX: 610-738-0437 fmonson-at-wcupa.edu CASI URL: http://darwin.wcupa.edu/casi/ WCUPA URL: http://www.wcupa.edu/ Visitors URL: http://www.wcupa.edu/_visitors/
} ---------- } From: Monson, Frederick C. } Sent: Friday, May 17, 2002 11:58 AM } To: 'List-Microscopy' } Subject: CPD Question Two } } ------------------------------------------------------------------------ } 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, } } } For those who order CO2-w/siphon tube for critical point drying. } } Do you order: } } the 'Research Grade' CO2 (-at-$300) or } } the standard grade CO2 (-at-$7)? } } Thanks, } } Fred Monson } } } Frederick C. Monson, PhD } Center for Advanced Scientific Imaging } Schmucker II Science Center } West Chester University } South Church Street and Rosedale } West Chester, Pennsylvania, USA, 19383 } Phone: 610-738-0437 } FAX: 610-738-0437 } fmonson-at-wcupa.edu } CASI URL: http://darwin.wcupa.edu/casi/ } WCUPA URL: http://www.wcupa.edu/ } Visitors URL: http://www.wcupa.edu/_visitors/ } }
At 11:58 AM -0400 5/17/02, Monson, Frederick C. wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Sounds like you have a flow rate problem something is constricting the flow of CO2 into the chamber. The chamber will get warm when you fill it (the CO2 in the syphon tank is at 18 C vs the chamber at 5 C). When you cool the chamber the CPD uses vented high pressure CO2 to cool the chamber (PV=nRT), but since there is a restriction in the flow from the CO2 supply tank, the CO2 back flows from the chamber dropping the CO2 liquid level.
I have found CO2 flow problems caused by:
- low CO2 supply tank
- tank valve must be openned fully (minus one 1/2 turn) - don't use the tank valve as a regulator.
- clogged filters. I have worked with different setups with various line filters (particle, oil, moisture, etc.) which get clogged and need replacing. I have also found some CPDs have (scintered?) metal mesh filters for particle filtration and these get clogged too.
- Worked with one instrument in which the internal plumbing lines were just too small and if you flushed or cooled too fast the liquid level in the chamber would drop and you had to be very carful and slow about things.
Hope it helps!
(Oh we use the cheap standard CO2)
On 16 May 2002, at 16:11, Monson, Frederick C. wrote:
} } Hi All, } We have a EMITech K850 Critical Point Dryer and a new tank of } Research Grade CO2, and we have problems. } The runs have all of a sudden become VERY inconsistent. } } Ambient temp in the Lab is around 18oC } After cooling the chamber to 5oC and opening the Inlet valve, the } pressure rises to 750psi at which is will remain for at least an hour with } all valves closed. } With the Inlet valve open, however, and waiting for liquid CO2 to } show in the sight glass, the temperature begins to rise and does so to } around 10oC at which point the fluid begins to rise in the glass to about } 1/8 of the 1cm diameter. } If I re-cool the chamber to 5oC, the fluid disappears. } If I wait for up to 3 minutes, one of two things happens. } 1. the fluid reappears and rises to 1/2 the sight window, } or } 2. I see nothing until I release the pressure and for a } brief period note the fluid level show at the very top of the sight glass } and fall and disappear very rapidly. } After the first run, which I cannot control, I cannot merely recyle } the unit. I have to wait an hour to demonstrate another unsatisfactory } test. } } If anyone can help me ferret out this poltergeist, I would be most } appreciative. I must say that I am convinced that I am dealing with a } daemon from the PChem lab.
If it is simply a matter of recirculation, it shouldn't be a problem even it there was a difference of several stories. Whether the pump is on the roof or in the EM room, since the inlet and outlet are at approximately the same height, there should be no net elevation head to be concerned about.
You would have the extra elevation head generating increased pressure in the line at its low point, but that it would only amount to about 15 psi or one bar for that height difference.
There may be some issue due to the length of the loop, but I will leave that to someone with more experience in that area.
Warren
At 12:11 PM 5/19/02 +0100, you wrote: } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America
Thanks to all who tried to help me with my head problem, I mean my microscope head problem ;-)
The guys from the company whose camera we bought came down and fixed the problem we were having with the camera. Now it looks like we're needing to buy a new LM, one that has the proper Trinoc head to handle our camera.
Again thanks to all who assisted me.
Looking at tiny things on big microscopes,
Paula :-)
Paula Sicurello George Washington Univ. Medical Center Dept. of Pathology, Ross Hall rm 505 Electron Microscope Lab 2300 Eye St. Washington, DC 20037 202-994-2930 phone 202-994-2518 fax
University of Connecticut Institute of Materials Science
Postdoctoral Positions
Two post-doctoral position are available immediately within the Institute of Materials Science at the University of Connecticut. Both positions require extensive hands-on experience in transmission electron microscopy, scanning electron microscopy, and x-ray diffraction. These positions are one-year appointments, with possible renewal for a second year.
The first position is for work on characterization and synthesis of ceramic coatings, thin films, and nanocomposites. Experience in the areas of materials chemistry and synthesis/processing is highly desirable. Contact: Prof. Nitin Padture at: nitin.padture-at-uconn.edu
The second position is for a study of the character and motion of interfacial defects in titanium aluminide alloys. An individual with prior experience in the use of HREM and analysis of interfacial crystallography would be preferred. Contact Prof. Mark Aindow at m.aindow-at-uconn.edu
To apply, please send a complete resume, together with a list of publications and contact details for 3 referees to the appropriate contact named above. Screening of applications will begin on June 1, and will continue until the positions are filled. We encourage applications from under-represented groups, including minorities, women and people with disabilities.
Mark Aindow, Associate Professor, Department of Metallurgy and Materials Engineering Institute of Materials Science, 97 North Eagleville Road, Unit 3136 University of Connecticut, Storrs, CT 06269-3136, USA
We are closing a Neurobiology EM lab and have an extra working Zeiss 902 available. If you are interested look at the official MSA website and the Surplus Listing.
Karen L. Bentley, M.S.(previously Jensen) Associate Scientist & Project Manager Electron Microscope Research Core University of Rochester Medical Center Rochester, NY 14642 585-275-1954
Chris, We have a Hitachi H7500, and a 3000-N. We use an air cooled Haskaris chiller for both, and located the chiller in a well ventilated rooftop service enclosure, approx. 12 metres above the EM room. In 2 years we have had no problems with this set-up. Saves water, eliminates noise and heat near the microscopes, plus the space savings.
David O'Neil Institute for Marine Biosciences National Research Council of Canada 1411 Oxford St. Halifax, NS B3H 3Z1 ph. 902-426-8258 fax 902-426-9413 david.o'neil-at-nrc.ca http://www.imb.nrc.ca/micros_e.html
-----Original Message----- } From: Chris Jeffree [mailto:c.jeffree-at-ed.ac.uk] Sent: May 19, 2002 8:11 AM To: microscopy-at-sparc5.microscopy.com
In about 6 months time I will have to move my microscopes into a newly re-furbished two-storey building. The chillers for the FEI CM120 and Hitachi 4700 may have to be located on the roof, at about 8.5 metres from ground level. I would like to hear from anyone who has considered this, and would particularly value the first-hand experiences of anyone who has already tried it. Are the pumps in standard chillers capable of dealing with an 8-metre head?
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I have a customer who needs to determine whether his glass and crystal objects were polished by hand or with machines. The objects are too big to fit in microscope, so I am looking for advice how to prepare replicas of their surfaces which will not leave marks on the objects.
Frederick C. Monson, PhD Center for Advanced Scientific Imaging Schmucker II Science Center West Chester University South Church Street and Rosedale West Chester, Pennsylvania, USA, 19383 Phone: 610-738-0437 FAX: 610-738-0437 fmonson-at-wcupa.edu CASI URL: http://darwin.wcupa.edu/casi/ WCUPA URL: http://www.wcupa.edu/ Visitors URL: http://www.wcupa.edu/_visitors/
} ---------- } From: kchamusco-at-mail.ifas.ufl.edu } Sent: Saturday, May 18, 2002 9:56 PM } To: Microscopy-at-sparc5.microscopy.com } Subject: Ask-A-Microscopist: corn pollen } } ------------------------------------------------------------------------ } 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 } -----------------------------------------------------------------------. } } } Below is the result of your feedback form (NJZFM-ultra-55). It was } submitted by (kchamusco-at-mail.ifas.ufl.edu) from } http://www.msa.microscopy.com/Ask-A-Microscopist.html on Saturday, } May 18, 2002 at 16:01:58 } -------------------------------------------------------------------------- } - } } Email: kchamusco-at-mail.ifas.ufl.edu } Name: karen chamusco } } Organization: U of FL } } Education: Graduate College } } Location: Gainesville FL } } Question: I'm sorry if I should be usinf the list serve but this is } the only page I could find to ask a question. I have been working } with corn pollen and trying to embed it in LR White resin for } immunolabeling in TEM. I thought I had this problem solved, but, } apparently I don't. When I get my pollen through the EtOH series up } to 95% it looks very good, but when I try to embed it in the resin it } collapses. I have tried putting it in resin/EtOH at 20% steps and } directly embedding it in 100% resin. The 20% stepwise series seems to } be the least destructive and I can get partially collapsed pollen } sometimes. I really need to be able to see inside a "fluffy" whole, } uncollapsed pollen grain. Is there anyone who can help with this } before I pull out the rest of my hair? If necessary to know, I fix } in 4% paraformaldehyde + 0.5% gluteraldehyde + 4% sucrose + 0.3% } tween {to get the samples to sink}. I vacuum infiltrate for 5 minutes } then I leave them in the fridge overnight. I then rinse with PBS and } send through a 10% EtOH series{anything greater causes the pollen to } collapse}. Then the rest is as I described above. Thanks, Karen } } -------------------------------------------------------------------------- } - } }
A conservator or scientists at the Corning Museum of Glass can advise you. Their main number is 800.732.6845.
James Martin Conservation Scientist
----- Original Message ----- } From: "Dusevich, Vladimir" {DusevichV-at-umkc.edu} To: "microscopylistserver" {Microscopy-at-sparc5.microscopy.com} Sent: Tuesday, May 21, 2002 1:45 PM
-- [ From: Garber, Charles A. * EMC.Ver #3.1 ] --
Vladimir Dusevich wrote: ============================================================ I have a customer who needs to determine whether his glass and crystal objects were polished by hand or with machines. The objects are too big to fit in microscope, so I am looking for advice how to prepare replicas of their surfaces which will not leave marks on the objects. ============================================================ We have done something very similar to this, the first time going back into the mid-1970's. We used what was then the prototype of the SPI Supplies : "Wet Replica Kit" as shown on URL http://www.2spi.com/catalog/spec_prep/wet_rep_kits.shtml
I realize this is not a wet surface but the kit was originally developed for the replication of a "wet" surface such as a plant leaf or even human skin.
Since it is a silicone, so long as the components are properly mixed, there should be no residue left behind on the surface. And the lift-off is easy enough that one does not generally need any kind of metal tools (e.g. a scalpel blade or tweezers) to help get the left off started.
We have also tried the cellulose acetate replica approach, see URL http://www.2spi.com/catalog/submat/cellulose-acetate-replicating-tape-sheets .shtml but we have had greater difficulty getting the cellulose acetate to lift off without the use of some kind of sharp instrument to start the lift-off.
Another advantage of the Wet Replica kit is that the replica itself can be replicated so that what goes into the SEM is something that spatially, looks just like the actual surface.
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 ######################## ============================================
We have a Leitz DMRBE OM and have just purchased a Leica DC 300F digital camera to use with it. The engineer recommended we get a x0.63 C-mount adaptor to use with the camera, particularly for fluorescence work "to concentrate the low light levels".
When using the camera with the x0.63 adaptor we get a dark shading on one side of the image(approximately 25% of the width of the image). This shading is independent of the camera alignment (ie you can rotate the camera and the shading doesn't rotate (although the image does)) and it also appears to be independent of the alignment of the adaptor. (ie you can rotate the adaptor and the shading doesn't rotate)
If you use a plain tube adaptor or a 1x adaptor there is no evidence of this shading. We have also tried the camera on other microscopes with identical results (ie shading only when using the x0.63 adaptor). We have also tried two different x0.63 adaptors and the shading was the same.
In the manual it mentions that some vignetting MAY occur using the x0.63 adaptor. Is this what we are seeing? The manual doesn't offer a solution other than not using the x0.63 adaptor. Does anyone have any ideas how we may be able to get around this problem other than not using the adaptor?
Thank you very much in advance.
Colin Veitch
Instrumentation Scientist Late Stage Innovation Group CSIRO Textile and Fibre Technology PO Box 21, BELMONT, Vic. 3216. Australia.
The information contained in this e-mail message may be privileged or confidential information. If you are not an intended recipient, you may not copy, distribute or take any action in reliance on it. If you have received this message in error, please telephone CSIRO Textile and Fibre Technology on +61 3 5246 4000.
I would like to offer you the opportunity to put your samples into our large chamber SEM. There is enough space for glass and crystal objects up to a volume of 1 cubic meter and 500 pounds of weight. Further more we can analyze the chemical composition of the glass surfaces by EDS.
Especially the analytic capabilities might be an advantage in distinguishing the production method.
email: mklein-at-visitec-em.de WWW: http://www.visitec-em.de ++++ Home of the world's largest SEM ++++
-----Ursprüngliche Nachricht----- Von: Dusevich, Vladimir [mailto:DusevichV-at-umkc.edu] Gesendet: Dienstag, 21. Mai 2002 19:45 An: microscopylistserver Betreff: Replicas of glass surface
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I have a customer who needs to determine whether his glass and crystal objects were polished by hand or with machines. The objects are too big to fit in microscope, so I am looking for advice how to prepare replicas of their surfaces which will not leave marks on the objects.
I have a user with the same basic need, only looking at marks on ancient ceramics. These are museum pieces and cannot be altered. He makes casts with latex or wax, usually latex.
Phil
} I have a customer who needs to determine whether } his glass and crystal objects were polished by hand } or with machines. The objects are too big to fit } in microscope, so I am looking for advice how to } prepare replicas of their surfaces which will not } leave marks on the objects. } } Thank you, } } Vladimir Dusevich
-- Philip Oshel Supervisor, BBPIC microscopy facility Department of Animal Sciences University of Wisconsin 1675 Observatory Drive Madison, WI 53706 - 1284 voice: (608) 263-4162 fax: (608) 262-5157 (dept. fax)
You use a .63x tube normally to adapt the field of view of the camera to the field of view through the binoculars. I am not sure what that has to do with "concentrating the light". And the physical reason behind that is, that the camera uses a chip that is bigger than the standard TV chips. Some vignetting (darker edges) is indeed normal when you use such a setup, but you may be able to minimize it by carfully adjusting all the parameters of the microscope and illumination path. In particular, it should be symmetric. Since you are using a digital camera, you can correct the images by using a shading or background correction. That's a software feature, and you may have to check if it is supported. If not, you can take a background image by removing the sample and taking a picture. then take a normal picture with your sample and divide or subtract the background image from the regular image.
mike
} } } } } } } } } } WE HAVE MOVED { { { { { { { { { please make a note of the new address below
Michael Bode, Ph.D. Soft Imaging System Corp. 12596 West Bayaud Avenue Suite 300 Lakewood, CO 80228 =================================== phone: (888) FIND SIS (303) 234-9270 fax: (303) 234-9271 email: mailto:info-at-soft-imaging.com web: http://www.soft-imaging.com ===================================
-----Original Message----- } From: "Colin.Veitch-at-csiro.au"-at-sparc5.microscopy.com [mailto:"Colin.Veitch-at-csiro.au"-at-sparc5.microscopy.com] Sent: Tuesday, May 21, 2002 11:46 PM To: microscopy-at-sparc5.microscopy.com
Hi All,
This question is on behalf of our OM operator.
We have a Leitz DMRBE OM and have just purchased a Leica DC 300F digital camera to use with it. The engineer recommended we get a x0.63 C-mount adaptor to use with the camera, particularly for fluorescence work "to concentrate the low light levels".
When using the camera with the x0.63 adaptor we get a dark shading on one side of the image(approximately 25% of the width of the image). This shading is independent of the camera alignment (ie you can rotate the camera and the shading doesn't rotate (although the image does)) and it also appears to be independent of the alignment of the adaptor. (ie you can rotate the adaptor and the shading doesn't rotate)
If you use a plain tube adaptor or a 1x adaptor there is no evidence of this shading. We have also tried the camera on other microscopes with identical results (ie shading only when using the x0.63 adaptor). We have also tried two different x0.63 adaptors and the shading was the same.
In the manual it mentions that some vignetting MAY occur using the x0.63 adaptor. Is this what we are seeing? The manual doesn't offer a solution other than not using the x0.63 adaptor. Does anyone have any ideas how we may be able to get around this problem other than not using the adaptor?
Thank you very much in advance.
Colin Veitch
Instrumentation Scientist Late Stage Innovation Group CSIRO Textile and Fibre Technology PO Box 21, BELMONT, Vic. 3216. Australia.
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Hi everybody - what is the best method for prep on a dried out moth? Just Au coat or if you have low vacuum mode available - go with that uncoated? Thanks Barb
How difficult will it be to get up on the roof to check the chillers for water level? I check mine weekly. Will the water lines freeze in the winter? Joyce Craig Chicago State University
1% Toluidine Blue O 1% Sodium Tetraborate Dodecahydrate 30% Ethanol in DDI
I've been using this stain for years on Epon-Araldite sections and Durcupan sections with no problems in getting satisfactory staining. When I have 30-50mL remaining, I always make a new batch so it's ready the next time I need it , but this time I forgot. I made a new solution and had to use it right away. I stained my sections as usual, but the color of the sections was bright blue instead of the more purple-blue we desire. Thinking that I'd made a mistake in preparing the solution, I made another batch and decided to wait overnight to try it, but again the sections were bright blue.
I was never aware of the need to do this, but does this solution need to "ripen" for a week or so before using? I can't think of any other reason. The quality of our water hasn't changed, and everything else is the same as I've always used.
Thank you for any help you can give me.
Jaclynn M. Lett, Research Technician Electron Microscopy Core Facility Fay and Carl Simons Center for Biology of Hearing and Deafness Central Institute for the Deaf 4560 Clayton Ave. St. Louis, MO 63110
You could try dental impression materials, available from any dental supplier. There are various types, I think the best type for your purpose would be one of the silicone-based ones. This would give a negative impression, of course. To get a positive I use epoxy resins: place the silicone impression at the bottom of a small container and pour a de-bubbled resin to make a layer 2 or 3 mm thick. After curing, the resin impression is indistinguishable from the original in the SEM. Hope this helps.
Lesley Weston.
on 21/05/2002 10:45 AM, Dusevich, Vladimir at DusevichV-at-umkc.edu wrote:
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } } I have a customer who needs to determine whether } his glass and crystal objects were polished by hand } or with machines. The objects are too big to fit } in microscope, so I am looking for advice how to } prepare replicas of their surfaces which will not } leave marks on the objects. } } Thank you, } } Vladimir Dusevich }
Butterlies and moths, and other scaly insects such as some beetles etc. can be a right pain. The overlapping scales make it almost impossible to put down a continuous coating. Even well-coated specimens may give problems with charging. If the whole moth is the objective, then the underside needs to be coated as well as the top. I contributed a tip for doing that with hard objects like seeds etc. some time ago, but the method I described then will damage a moth. The simplest thing to do with a moth is to coat the underside before mounting. Once mounted coat the top. The more angles you coat from the better, so rotary coating will help, even in a sputter coater. Carbon seems to reach the parts other coating materials cannot reach, so a preliminary rotary/tilting coating with carbon before sputtering may improve the overall conductivity. I used to do that routinely, but it has gone out of favour, mostly for good reasons. Low vac mode may help somewhat, but not if you need high res images of scale details. Keep the kV and beam current as low as possible, use short exposures if you have enough signal to do so. In the worst-case scenario collecting an image by frame-integration at tv rate may be the only way, but image quality is rarely very good. Try a little specimen bias if available. Use a FEG SEM if available. Use the lower detector if there is a choice.
Chris
} ----- Original Message ----- } From: "barbara maloney" {bmalon01-at-fiu.edu} } To: "'microscopy-at-msa.microscopy.com'" } {microscopy-at-sparc5.microscopy.com} } Sent: Wednesday, May 22, 2002 3:10 PM } Subject: SEM technique } } } } -------------------------------------------------------------------- } ---- } } 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 everybody - what is the best method for prep on a dried out moth? } } Just Au coat or if you have low vacuum mode available - go with that } } uncoated? } } Thanks } } Barb } } } } }
If specimen permits, I always coat it. Images are much better for coated specimens.
Vladimir
} -----Original Message----- } From: barbara maloney [mailto:bmalon01-at-fiu.edu] } Sent: Wednesday, May 22, 2002 9:10 AM } To: 'microscopy-at-msa.microscopy.com' } Subject: SEM technique } } } -------------------------------------------------------------- } ---------- } 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 everybody - what is the best method for prep on a dried out moth? } Just Au coat or if you have low vacuum mode available - go with that } uncoated? } Thanks } Barb } } }
Would any one please share with use your user fees of your microscopic facility including charges for imaging? I would appreciate your help. We are in the process of establishing such charges and hope to find willingness of your part to share this information.
Many thanks.
Anne-Marie Brun Research Associate Mol. Biology and Genetics UNT HSC Fort Worth, Texas
I have an update to my hotspot problem that unfortunately does not include any solutions.
First of all, we don't get the problem on the transmitted side of the scope. The cheap halogen lamp seems to work fine. Also, we have another Nikon TE300 microscope in the lab with the same Coolsnap HQ camera and we get exactly the same thing. That seems rather suspicious.
I think I can see this effect with a regular video camera if I threshold the image.
Here is a list of things we have done so far. None of them have produced any appreciable change.
1) 10 degree holographic diffuser in place of one of the neutral density filters right after the lamp. 2) IR filter in the collector lens. 3) IR filter before the camera. 4) aligned and misaligned the lamp in every possible way. 6) focused and defocused the lamp in every possible way. 7) changed out filter block. 8) reduced the exposure time of the camera down to 1 ms.
So it doesn't seem to be IR.
I'll let you know if we figure it out.
Eric
Eric Johnston Design Engineer and Research Specialist Department of Bioengineering University of Pennsylvania 5170 Vagelos 220 South 33rd Street Philadelphia, PA 19104 215-573-6696 215-573-7616 (F) 215-573-2071 ericdj-at-seas.upenn.edu
You should be aware, as should anyone else who might attempt this, that certain glass and rock crystal artifacts are prone to catastrophic fracturing when subjected to pressure or humidity changes - crystal in the first case and glass in the second.
Rock crystal artifacts are often subject to considerable residual stress and must be protected from sudden temperature or pressure excursions. Certain glasses, many from archaeological origins but also some from the 19th Century, are unstable with respect to water and may have undergone partial hydrolysis with a resulting incorporation of hydrous silica in places formerly occupied by alkali-oxygen-silica links. Such glasses are sometimes visually unchanged but may shatter to powder when subjected to dehydrating conditions as under the vacuum of a SEM chamber.
While the advantages of your large chamber instrument are well known, the examination of replicas is safer unless a great deal is known about the behavior of the specific object.
John Twilley Art Conservation Scientist
On Wed, 22 May 2002 09:39:39 +0200 Martin Klein {Visitec-at-t-online.de} wrote:
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Dear Vladimir,
I would like to offer you the opportunity to put your samples into our large chamber SEM. There is enough space for glass and crystal objects up to a volume of 1 cubic meter and 500 pounds of weight. Further more we can analyze the chemical composition of the glass surfaces by EDS.
Especially the analytic capabilities might be an advantage in distinguishing the production method.
email: mklein-at-visitec-em.de WWW: http://www.visitec-em.de ++++ Home of the world's largest SEM ++++
-----Ursprüngliche Nachricht----- Von: Dusevich, Vladimir [mailto:DusevichV-at-umkc.edu] Gesendet: Dienstag, 21. Mai 2002 19:45 An: microscopylistserver Betreff: Replicas of glass surface
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I have a customer who needs to determine whether his glass and crystal objects were polished by hand or with machines. The objects are too big to fit in microscope, so I am looking for advice how to prepare replicas of their surfaces which will not leave marks on the objects.
Try perhaps to control the pH of your Toluidine Blue stain solution.
If I remember well, Toluidine Blue Stain is metachromatic when it is acidic (no real difference between pH 4 and 7) but it is no more (only blue) when basic (for example at pH 8.2, at least for plant tissue embeded in JB4).
Hope it helps !
Chris Wuethrich Beth Israel Deaconess Medical Center 330 brookline AVE Boston, MA 02215 cwuethri-at-caregroup.harvard.edu
In a message dated 05/21/2002 11:02:03 PM US Mountain Standard Time, Colin.Veitch-at-csiro.au-at-sparc5.microscopy.com writes:
{ { When using the camera with the x0.63 adaptor we get a dark shading on one side of the image(approximately 25% of the width of the image). This shading is independent of the camera alignment (ie you can rotate the camera and the shading doesn't rotate (although the image does)) and it also appears to be independent of the alignment of the adaptor. (ie you can rotate the adaptor and the shading doesn't rotate) } }
Colin,
I know the Leica DC500 has a "shading correction" routine you can use to even out the illumination, but I don't know if the 300F has the same routine. We had a similar problem with a 0.63X adapter on a DC500, and running the "shading correction" took care of the problem.
If the camera can do this (check the manual), you will see a "shading" function on the left side of the screen where you set the image size, auto contrast, etc. Proceed as follows:
Click on "shading" and first set the black level: shut off all light to the camera and click on "black level." After this, click on "shading" again and then set the white level by sending light to the camera and making sure there is no specimen or tissue in the field of view. Then, grab a "white level." You may have to play with the "brightness" slider at the top of the window until the camera accepts the bright level. It will inform you if the illumination is too dark or too light.
Also, when you set the white level you will have to assign a name to it...you can call it "10x," or "40x," or whatever, for the objective you are using, or maybe "brightfield" or another name of your choice.
If you have access to this routine on the 300F, it should take care of moderate differences in illumination such as hot spots and shadows.
If the shading is severe, it may be too much for the correction factor to handle. If this is the case, you will probably either need to use a 1.0X adapter or a Leica c-mount "vario-zoom" adapter, which allows you to set the magnification from about 0.3 up to 1.3 or so, much like a zoom lens for a 35mm camera.
Hi everybody - thanks to those who responded. Wanted to let you know, we ended (before I received your responses) coating 367 Ang of Au for 2 min. Prior to coating we did view at low vacuum with no coat - got an image, of course not as nice as when we coated at high vacuum. Just used a large carbon tab on viewed ventral side of moth - really nice images. Thanks gang. Barb P.S. I will try your suggestions. Thanks again
} ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.Com } On-Line Help http://www.msa.microscopy.com/MicroscopyListserver/FAQ.html } -----------------------------------------------------------------------. } } Hi everybody - what is the best method for prep on a dried out moth? } Just Au coat or if you have low vacuum mode available - go with that } uncoated? } Thanks } Barb
Hi Barb I routinely deal with insects especially hairy and scaly specimens. What I have found is, firstly when you mount the specimen - I always mount the whole animal on a pin - use carbon or silver impregnated glue to stick the moth onto the pin or directly onto a stub. Secondly if mounting directly onto an aluminum stub, I use a double sided carbon sticky tab on the stub then apply the glue to the tab then the specimen. This ensures good conductivity. Thirdly when coating be careful not the coat too heavily with gold - you will loose some fine detail on the scales, antennae etc. Coat the specimen several times (short coating times) in differing positions - this will ensure total coverage. With the specimen on a pin it makes coating the whole specimen a lot easier. Once coated I then recoat the pin with the carbon glue. This makes the pin nonconductive and once in the SEM you do not see the pin. Thus the moth looks like it is sitting in space.
We use a LEO 435VP SEM in high vacuum mode to do this work. The way I avoid charging (if it is charging much at all) is to use the Robinson Backscatter Detector. The images derived are fantastic. Quite contrasty!!! Another thing is I often mix the Backscatter signal with the Secondary signal. This allows me to enhance the background, bring out the edges, seta etc that appear to be flattened in the backscatter image.
I hope this helps
Sue
-- Sue Lindsay
SEM Laboratory Manager Scanning Electron Microscope Unit The Australian Museum 6 College st Sydney, 2010 NSW, Australia
} ------------------------------------------------------------------------ } 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 everybody - what is the best method for prep on a dried out moth? } Just Au coat or if you have low vacuum mode available - go with that } uncoated? } Thanks } Barb
Hi Barb I routinely deal with insects especially hairy and scaly specimens. What I have found is, firstly when you mount the specimen - I always mount the whole animal on a pin - use carbon or silver impregnated glue to stick the moth onto the pin or directly onto a stub. Secondly if mounting directly onto an aluminum stub, I use a double sided carbon sticky tab on the stub then apply the glue to the tab then the specimen. This ensures good conductivity. Thirdly when coating be careful not the coat too heavily with gold - you will loose some fine detail on the scales, antennae etc. Coat the specimen several times (short coating times) in differing positions - this will ensure total coverage. With the specimen on a pin it makes coating the whole specimen a lot easier. Once coated I then recoat the pin with the carbon glue. This makes the pin nonconductive and once in the SEM you do not see the pin. Thus the moth looks like it is sitting in space.
We use a LEO 435VP SEM in high vacuum mode to do this work. The way I avoid charging (if it is charging much at all) is to use the Robinson Backscatter Detector. The images derived are fantastic. Quite contrasty!!! Another thing is I often mix the Backscatter signal with the Secondary signal. This allows me to enhance the background, bring out the edges, seta etc that appear to be flattened in the backscatter image.
I hope this helps
Sue
-- Sue Lindsay
SEM Laboratory Manager Scanning Electron Microscope Unit The Australian Museum 6 College st Sydney, 2010 NSW, Australia
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A student working in the lab is interested in using TEM to examine thickness of the chitinous exoskeleton and the interface between muscle and skeletal attachments in some insects (Heteroptera). Does someone have experience in embedding and ultramicrotomy of this type of material? I expect we will have some problems with the harder parts pulling out of the resin. Are there any tricks we should know about? Any special fixation steps or suggestions? Thanks.
Marie
Dr. Marie E. Cantino Dept. of Physiology and Neurobiology, U-2242 University of Connecticut Storrs, CT 06269-2242 Phone: 860-486-3588 Fax: 860-486-6369
} Morning Anne-Marie, } When I need such information, I try searching Google for {core } facility charges} . Pages and pages. } } Regards, } } Fred Monson } } Frederick C. Monson, PhD } Center for Advanced Scientific Imaging } Schmucker II Science Center } West Chester University } South Church Street and Rosedale } West Chester, Pennsylvania, USA, 19383 } Phone: 610-738-0437 } FAX: 610-738-0437 } fmonson-at-wcupa.edu } CASI URL: http://darwin.wcupa.edu/casi/ } WCUPA URL: http://www.wcupa.edu/ } Visitors URL: http://www.wcupa.edu/_visitors/ } } } } ---------- } From: Anne-Marie Brun } Sent: Wednesday, May 22, 2002 3:38 PM } To: Microscopy-at-sparc5.microscopy.com } Subject: Microscopic user fees } } ------------------------------------------------------------------------ } The Microscopy ListServer -- Sponsor: The Microscopy Society of America } To Subscribe/Unsubscribe -- Send Email to ListServer-at-MSA.Microscopy.