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From: DUNHAMDJ-at-uwec.edu
Date: Wed, 2 Jan 2008 11:09:00 -0600
Subject: [Microscopy] Electron Microscopist Position

Contents Retrieved from Microscopy Listserver Archives
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James,
Have you looked at "operating microscopes"? Although binocular (stereo),
they generally have very long working distances. I have an old Zeiss
dissecting scope with a focal length in the range of 200mm. I love it,
although there are certainly issues on resolution at 40X. I mostly use it
at 6X.

Ken Converse
owner

QUALITY IMAGES
Servicing Scanning Electron Microscopes
Since 1981
474 So. Bridgton Rd.
Bridgton, ME 04009
207-647-4348
Fax 207-647-2688
kenconverse-at-qualityimages.biz
qualityimages.biz



-----Original Message-----
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Sent: Monday, December 31, 2007 11:47 AM
To: kenconverse-at-qualityimages.biz

This Question was submitted to Ask-A-Microscopist by (james99-at-uab.edu) from
http://www.microscopy.org/Ask-A-Microscopist/Ask-A-Microscopist.html
on Wednesday, December 19, 2007 at 13:52:08
Remember to consider the Grade/Age of the student when considering the
Question
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Please reply to both james99-at-uab.edu as well as to the Microscopy
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Email: james99-at-uab.edu
Name: James Borham

Organization: University of Alabama at Birmingham

Education: Undergraduate College

Location: Birmingham, Alabama, United States of America

Title: Finding a Specialized Microscope

Question: I'm trying to find a new microscope with some specialized
features, and I'm having a lot of trouble. I'm hoping one of you may
be able to help me out.
The feature that is needed most, and has been impossible to find, is
a non-stereo microscope and/or lens with a parfocalizing distance of
90 mm or more.
Do you have any idea where I could find such a thing? Is a device
with such a long parfocalizing distance even classified as a
microscope?
I would appreciate any help on this problem.

---------------------------------------------------------------------------

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Analytical Scientist/Electron Microscopist

The University of Wisconsin Eau Claire is seeking applicants for an Analytical Scientist/Electron Microscopist in the Materials Science Center, an interdisciplinary analytical facility, specializing in materials characterization. This is a full-time professional academic staff position beginning as early as July 1st 2008. Potential applicants may obtain a complete position description and application requirements at www.uwec.edu/Matsci/EMposition.html. Women, minorities, individuals with disabilities and veterans are encouraged to apply. The University is responsive to the needs of dual career couples. Criminal background checks are required prior to employment.




------------------------------------------------------------------------
Dr. Doug Dunham
Director, Materials Science Center
University of Wisconsin Eau Claire
105 Garfield Avenue
Eau Claire, WI 54701
715-836-5312 fax: 715-836-3955
dunhamdj-at-uwec.edu



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From: cammer-at-aecom.yu.edu
Date: Wed, 2 Jan 2008 13:48:25 -0600
Subject: [Microscopy] Re: Re: MRI ? on maize embryos

Contents Retrieved from Microscopy Listserver Archives
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}
} Have a look at the website of The Microscience Group:
}
} http://www.microsciencegroup.com/

http://www.microsciencegroup.com/products_microimager.htm

This looks just like a system I saw at Harvard in May 1994 for
imaging lung with asbestos or other fibers for 3D reconstruction
using VoxelView running on an SGI.

-mc

____________________________________________________________________________
Michael Cammer Analytical Imaging Facility Albert Einstein Coll. of Med.
URL: http://www.aecom.yu.edu/aif/


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From: randerson20-at-tampabay.rr.com
Date: Wed, 2 Jan 2008 15:01:50 -0600
Subject: [Microscopy] January 2008 Microscopy Today Table of Contents

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Listers,

Here is the January 2008 Microscopy Today table of contents. I will
close the subscription list for this issue on Tuesday January 8, 2008.

Microscopists in North America and MSA members anywhere qualify for free
subscriptions. Anyone else may subscribe for US$60 per year (to
PARTIALLY cover postage). All subscriptions at
http://www.microscopy-today.com .

Thank you,
Ron Anderson, Editor
========================
Microscopy Used to Discover New, Cool Mineral!
Stephen W. Carmichael1, Mayo Clinic

Material Contrast of Scanning Electron and Ion Microscope Images of Metals
T. Suzukia*, M. Kudo*, Y.Sakai*, and T. Ichinokawa**, *JEOL Ltd.,
Akishima, Tokyo, **Waseda University, Tokyo, Japan

Effective Cell Identification and Segmentation in Fluorescence
Microscopy with New Fluorescent Whole Cell Stains
Suk J. Hong, Richik N. Ghosh, Thermo Fisher Scientific Inc., Rockford, IL

Giving your SEM or FIB a Helping Hand
Neil Rowlands, Oxford Instruments, Concord, USA, Gavin Frayne, Kleindiek
Nanotechnik, Tubingen, Germany, Bo Svarrer Hansen, Capres A/S, Lyngby,
Denmark

An Introduction to 3D Microscopy Techniques
Megan MacNeil and Duncan McMillan, Carl Zeiss MicroImaging, Inc.
Thornwood, NY.

Scanning Transmission Electron Microscopy for Critical Dimension
Monitoring in Wafer Manufacturing
Haifeng Wang*, Jason Fang*, Jason Arjavac**,Rudy Kellner**, *Western
Digital Corporation, Fremont, CA, **FEI Company, Hillsboro, OR

Nanoelectromechanics of Inorganic and Biological Systems: From
Structural Imaging to Local Functionalities
B. J. Rodriguez,1,2 S. V. Kalinin,1,2 S. Jesse,1 G. Thompson,3 A.
Vertegel,3 S. Hohlbauch,4 R. Proksch4 ,1Mat. Sci. & Tech, and 2Ctr. for
Nanophase Matl. ORNL, Oak Ridge, TN, 3 Clemson University, SC, 4Asylum
Research, Santa Barbara, CA

Spatial Resolution in ACOM–What Will Come After EBSD
R.A. Schwarzer, Kappstr. 65, D-71083 Herrenberg, Germany

Lab-Tek Chamber Slide for TEM Prep: A Simple, Rapid, and Reliable
Protocol for In Situ Embedding Monolayer Cell Cultures in Epoxy and LR
White Resin
Gang Ning, Penn State University, State College, PA

Imaging Carbon Nanoparticles in Cells
Mhairi Gass* & Alexandra Porter**, *SuperSTEM, Daresbury Lab.,
Daresbury, **Imperial College London, London, U.K.

Automatic Acquisition and Image Analysis of 2D Crystals
N. Coudray*, F. Beck**, J.-L. Buessler*, A. Korinek**, A. Karathanou*,
H. Rémigy***, H. Kihl*, A. Engel***, J.M. Plitzko**, J.-P. Urban*,
*Université de Haute Alsace, Mulhouse, France, **Max Planck Inst.
Martinsried, Germany, ***University of Basel, Switzerland

Industry News

NetNotes
SAMPLE PREPARATION - osmium ignition
SAMPLE PREPARATION – wood for TEM
SAMPLE PREPARATION - perchloric acid hazards
SAMPLE PREPARATION - differential polymer staining
MICROTOMY - alternative ultramicrotome knives
IMAGE ANALYSIS - stitching high-resolution microscope images
IMMUNOCYTOCHEMISTRY – adherent cells
IMMUNOCYTOCHEMISTRY - pre-embedding tissue cultures
TEM: Objective aperture vs. EFTEM
TEM – alignment problem
TEM - lattice fringes
TEM - micelle solutions
TEM - ice contamination
EDX - plants and seeds
EDX - biological sample

Dear Abbe

Advertiser's Index


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From: sau_silwal-at-yahoo.com
Date: Wed, 2 Jan 2008 15:16:11 -0600
Subject: [Microscopy] Re: Embedding pine needles in JB-4

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi,

Happy New Year!!

Has anyone embedded pine needles in JB-4 and sectioned
for LM? I had problem with orientation when I used
plastic beem capsules before. I have been trying
silicon rubber molds under 10psi. But it doesn't
polymerize competely. What is the max psi i can go not
to damage both tissue and plastic.
I have been also thinking of switching to LR-white.
But I dont know if i get better result. I would
appreciate any kind of advice on this.

Thanks.

Sau Silwal


Send instant messages to your online friends http://uk.messenger.yahoo.com

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From: sau_silwal-at-yahoo.com
Date: Wed, 2 Jan 2008 15:16:51 -0600
Subject: [Microscopy] Re: Embedding pine needles in JB-4

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi,

Happy New Year!!

Has anyone embedded pine needles in JB-4 and sectioned
for LM? I had problem with orientation when I used
plastic beem capsules before. I have been trying
silicon rubber molds under 10psi. But it doesn't
polymerize competely. What is the max psi i can go not
to damage both tissue and plastic.
I have been also thinking of switching to LR-white.
But I dont know if i get better result. I would
appreciate any kind of advice on this.

Thanks.

Sau Silwal


Send instant messages to your online friends http://uk.messenger.yahoo.com

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7, 19 -- Subject: Re: Embedding pine needles in JB-4
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From: baskin-at-bio.umass.edu
Date: Wed, 2 Jan 2008 15:44:24 -0600
Subject: [Microscopy] Re: Embedding pine needles in JB-4

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Sau,
Not sure exactly if this will solve your problem, but for
what its worth, you can get capsules that are like BEEMs except that
they have a completely flat bottom. They are made by TAAB but
available from major supply houses (no finanical connection). This
gives a nice 7 mm (or so) flat surface. You can also get this out of
a standard BEEM by flipping it upside down, although you have to mess
about to keep the resin from leaking (definitely a mess, but possible
to do).

Hope this helps,
Tobias

}
} Hi,
}
} Happy New Year!!
}
} Has anyone embedded pine needles in JB-4 and sectioned
} for LM? I had problem with orientation when I used
} plastic beem capsules before. I have been trying
} silicon rubber molds under 10psi. But it doesn't
} polymerize competely. What is the max psi i can go not
} to damage both tissue and plastic.
} I have been also thinking of switching to LR-white.
} But I dont know if i get better result. I would
} appreciate any kind of advice on this.
}
} Thanks.
}
} Sau Silwal
}

--
_ ____ __ ____
/ \ / / \ / \ \ Tobias I. Baskin
/ / / / \ \ \ Biology Department
/_ / __ /__ \ \ \__ 611 N. Pleasant St.
/ / / \ \ \ University of Massachusetts
/ / / \ \ \ Amherst, MA, 01003
/ / ___ / \ \__/ \ ____
http://www.bio.umass.edu/biology/baskin/
Voice: 413 - 545 - 1533 Fax: 413 - 545 - 3243

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From: oshel1pe-at-cmich.edu
Date: Thu, 3 Jan 2008 09:00:55 -0600
Subject: [Microscopy] Re: MRI ? on maize embryos

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Sorry for the late reply, but you might contact Jamie Weichert at UW-Madison:
http://www.radiology.wisc.edu/research/contrastAgentLab/index.php

He works on this sort of problem for both MRI and microCT.
The issue is more likely, can the instruments get the resolution you
need? But I suspect they can.

Phil

}
} Daar coleagues
} I am working on a project on the vascular puncture inoculation
} (VPI) of maize viruses into maize embyos. We need to have a 3-D
} picture of the vascular bundles in (germinating) maize embyos, and a
} colleage of mine suggested MRI as a possible means to achieve that.
} I wonder if anyone has tried MRI on plants/ plant tissues, or if
} someone can suggest another more suitable method (apart from
} LM-serial sectioning). Thanks and Happy New Year to everyone.
}
}
} El-Desouky Ammar, Ph.D.
} Dept. of Entomology, OSU,
} 019 Selby Hall,
} OARDC, Wooster, OH 44691
} Tel: 330-263-3830.
} FAX: 330-202-3563.
--
Philip Oshel
Microscopy Facility Supervisor
Biology Department
024C Brooks Hall
Central Michigan University
Mt. Pleasant, MI 48859
(989) 774-3576

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From: max_atena_parthenos-at-alice.it
Date: Thu, 3 Jan 2008 09:02:43 -0600
Subject: [Microscopy] viaWWW: Disposable microtome blades

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Email: max_atena_parthenos-at-alice.it
Name: Massimo

Organization: Private

Title-Subject: [Filtered] Disposable microtome blades

Question: Hi all,

I am an amateur naturalist.
I have made by myself a microtome and I also use to honing the blade with results quite good. Now I am testing a disposable blade. It was a kindly gift of a friend of mine who works in an histology laboratory.
I wonder where could I find disposable blades because it seems they are working well . Otherwise it is quite difficult to make and honing a blade by myself.
Does anybody know a factory that produces such kind of blades?
Any suggestions would be greatly appreciated.

Thank You.
Massimo


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From: Jill.Verlander-at-medicine.ufl.edu
Date: Thu, 3 Jan 2008 09:03:02 -0600
Subject: [Microscopy] viaWWW: coolwell chiller help

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Email: Jill.Verlander-at-medicine.ufl.edu
Name: Jill Verlander Reed

Organization: University of Florida

Title-Subject: [Filtered] coolwell chiller help

Question: Dear Listservers -

We returned to work today after a hiatus since 12/21. The afternoon before we shut down the lab for Christmas break, we turned off the scopes and chillers. All was well with the equipment before that.

Today, we tried to get everything going again, but the old Coolwell chiller (model S-075W) on our Zeiss EM10 is not working properly. When we tried to run it, there was no flow and the HiTemp warning light on the front panel was lit. This is supposed to shut off the system if the temp rises above 93 degrees F, which it is not (room temperature is 73 degrees, coolant temp about 71 degrees F). However, the "reset" switch on the P6 high temperature safety control box had not popped out.

If you turn the unit on and press the button (S-3) that bridges the high temperature limit control, and have the unit pumping only on itself (a short loop from supply to return), the pump runs normally. Intermittently, it will run normally either on "bypass" (which does not allow the compressor to come on) or on "normal" function. The compressor will come on when the unit is working and set on "normal." However, the unit will spontaneously shut down, and when it does, the hi temperature light comes on.

The compressor is cooled by house tap water: the supply and return lines are open and flowing. The coolant tank is full, magnetic float switch floating, and the filter looks okay - not pristine, but only slightly gray. We did have a "heat event" according to an unrelated computer that was left on during the break, but I don't see how that could have affected the chiller, since it was shut off at the time.

Does anybody have any suggestions as to what might be causing this problem and how to correct it?

Many thanks, and Happy New Year to all!

Jill Verlander Reed
University of Florida
College of Medicine Electron Microscopy Core Facility


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From: jeff-at-tss-consulting.com
Date: Thu, 3 Jan 2008 09:04:08 -0600
Subject: [Microscopy] viaWWW: Employment Opportunity

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Email: jeff-at-tss-consulting.com
Name: Jeff West

Organization: TSS Consulting Ltd.

Title-Subject: [Filtered] Employment Opportunity

Question: TRANSMISSION ELECTRON MICROSCOPY (TEM) TECHNICIAN or ENGINEER


Located on the MA/NH border 35 minutes from Boston, an exciting opportunity exists for an experienced TEM We are looking for a Technician or Engineer to join a team of scientists researching and developing materials for the semiconductor industry.
Working closely with the companyís TEM scientist, you will both prepare semiconductor materials for TEM (utilizing a T-tool and wedge technique) and be responsible for imaging of these samples with a JEOL 2100 TEM system.

A minimum of 3 years experience with TEM sample prep and imaging is required. Preference is for candidates with Materials Science or Engineering degrees (BS or MS).


For further information and to apply for this position please contact:
Jeff West
TSS Consulting, Ltd.
(877) 489-2425
Resumes may be sent to: jeff-at-tss-consulting.com



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From: susan.trant-at-viha.ca
Date: Thu, 3 Jan 2008 09:04:46 -0600
Subject: [Microscopy] AskAMicroscopist: EM film 5302

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This Question was submitted to Ask-A-Microscopist by (susan.trant-at-viha.ca)
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Email: susan.trant-at-viha.ca
Name: Susan Trant

Education: Graduate College

Location: Victoria, British Columbia, Canada

Title: EM film

Question: Hello everyone

I purchased Eastman Fine Grain Release Positive Film 5302 from Electron Microscopy Sciences for my TEM. The film is much thicker than the current product that I am using. I contacted some photo experts and they said that I needed a product called Dektol for a film developer.(Kodak) Does anyone use this film and if so, what developer do you use and what temperature and length of time for processing? The photography shop that I talked to also said that you do not dilute the stock solution before use.
We are receiving a new digital imaging system within the year.

Thanks

Sue Trant
EM Technologist
Vancouver Island Health Authority
Victoria, British Columbia,
Canada


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From: connellyps-at-nhlbi.nih.gov
Date: Thu, 3 Jan 2008 10:41:05 -0600
Subject: [Microscopy] Re: AskAMicroscopist: EM film 5302

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Sue,

I trashed my files on this film about six months ago thinking that I'd never
need to consult it again. There are several things that I do remember that
may be of interest to you. The following is from a 25 year old memory!

This film is quite good for TEM and the sheet film is thick also. You will
need to do an exposure test to see what gives the best results. If you have
an older scope you should be able to change the exposure time. Do several
times of the same area.

Keep film away from light! I used a very dark red filtered light that was
so dark that it was nearly useless even after giving my eyes time to adjust.
To load the film both into the scope camera holder and into the developing
tank I would turn my back to the light and load in front of me.

Dektol seems correct as the developer. I do not remember diluting it - try
using it straight from the stock solution that you make from the powder.
Adjust the temperature before turning out the room light. Try hot water
around a beaker with the developer in it and stir gently with the
thermometer.
I used a brown gal. bottle to store the developer, kept in the darkroom for
a month or so with no problems as to age. Just make sure the bottle is
stoppered well. If the developer starts to turn brown it is time to make up
a new batch. I think the temperature for making the developer is much hotter
than the film developing temperature so make sure you make it up with enough
time to cool before you want to use it.
(Stoppers work better than caps in my opinion)

Four minute development stands out in my mind; agitated several times. I
used the old apron type from Kodak to do the loading but any standard 35 mm
developing tank should work well. Make positive that you do not have any
bubbles stuck to the film by banging the tank on a counter surface a few
times after the developer is in the tank with the film.
Water rinse twice.
Kodak Rapid fixer 4 min. with agitation several times
Wash in running for 30 min.
Photoflo rinse for 15 sec.
Hang to dry with a weight on the bottom (to eliminate curling)

I used the film without perforations (holes along the sides). This
increased the area of the image greatly. If you do have a camera that can
use this film and have a negative holder that you can spare, find a shop
that can make the viewing holes of the holder larger by a few mm. If
scanning into a computer there will be no problem.

Hoping my recollections are accurate,
Pat

Patricia Stranen Connelly
NHLBI Electron Microscopy Core
National Institutes of Health
14 Service Road South
Bldg. 14E ­ Rm. 111B MSC 5570
Bethesda, MD 20892-5570
Phone 301-496-3491
connellyps-at-mail.nih.gov


} ----------------------------------------------------------------------------
} Email: susan.trant-at-viha.ca
} Name: Susan Trant
}
} Education: Graduate College
} Location: Victoria, British Columbia, Canada
} Title: EM film
}
} I purchased Eastman Fine Grain Release Positive Film 5302 from Electron
} Microscopy Sciences for my TEM. The film is much thicker than the current
} product that I am using. I contacted some photo experts and they said that I
} needed a product called Dektol for a film developer.(Kodak) Does anyone use
} this film and if so, what developer do you use and what temperature and length
} of time for processing? The photography shop that I talked to also said that
} you do not dilute the stock solution before use.
} We are receiving a new digital imaging system within the year.
}
} Thanks
}
} Sue Trant
} EM Technologist
} Vancouver Island Health Authority
} Victoria, British Columbia,
} Canada

} ==============================End of - Headers==============================



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From: dhitrys-at-qimaging.com
Date: Thu, 3 Jan 2008 11:54:33 -0600
Subject: [Microscopy] Webinar on Quantitative Fluorescence Imaging

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You are invited to attend a live, interactive, web-based instructional
seminar:

==========================================================
"Quantitative Image and Data Acquisition for Fluorescent Specimens"
Advice from a Facility Director

Presented by Brian Matsumoto, Ph.D., University of California, Santa Barbara
==========================================================

Details are below. Connection lines are limited so reserve yours now. There
is no charge to participate in this on-line seminar.


When:
=====================
Monday, 7-January, 1:30PM (New York time; 10:30 AM California time.)
Duration: Approximately 1 hour.

Pre-register (required) at:
http://magbiosystems.com/education/


Details:
=====================

Attendees will learn about issues affecting the quantitative accuracy of
fluorescence images acquired through a microscope and will pick up tips and
suggestions for improving image quality, making better use of the camera's
light collection abilities, and will learn the nomenclature associated with
digital imaging. Attendees will leave with a better understanding of how to
characterize and optimize their optical system, camera, and software. Bring
your questions to this live, interactive web-based seminar.

- What is bit depth and when/why does it matter?
- What is dynamic range?
- Characterizing your camera's linear range.
- Noise and other sources of data uncertainty.
- Maximizing your camera's light collection capabilities.
- Setting the best exposures.
- Correcting for photobleaching.
- Collecting images in 3D.


About the presenter
=====================
Brian Matsumoto, Ph.D. is the Director of the Integrated Microscopy Facility
and is an Associate Adjunct Professor for the department of Molecular,
Cellular and Developmental Biology Department at the University of
California Santa Barbara. He is the author of "Basic Methods in Light
Microscopy" (Cambridge University
Press) and editor of "Cell Biological Applications of Confocal Microscopy"
(Academic Press).


More instructional webinars are also shown at
http://magbiosystems.com/education
Register for any session of interest and feel encouraged to pass this along
to your colleagues.

Sponsored by the Microimaging Applications Group (MAG), a group of
independent imaging companies working cooperatively to provide an
unparalleled range of solutions for microimaging applications.

This seminar requires that attendees use a Java-enabled browser with a high
bandwidth connection. Audio is via toll-free telephone.

There is no charge to participate in this or the other on-line seminars.

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From: samuel.connell-at-stjude.org
Date: Thu, 3 Jan 2008 13:57:47 -0600
Subject: [Microscopy] viaWWW: Imaging Scientist

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Email: samuel.connell-at-stjude.org
Name: Samuel Connell

Organization: St. Jude Childrenís Research Hospital

Title-Subject: [Filtered] Imaging Scientist ñ St. Jude Childrenís Research Hospital

Question: Imaging Scientist ñ St. Jude Childrenís Research Hospital.

Currently, St. Jude Childrenís Research Hospital has an opening for an Imaging Scientist (Job Number 17216) in the Cellular Imaging Department.

The successful candidate would be responsible for assisting faculty, postdoctoral researchers, staff, and collaborators in advance microscopy techniques and methodologies, including laser scanning and spinning disk confocal fluorescence microscopy, wide-field microscopy, live cell imaging, FRET, FLIM, FRAP and TIRF, as well as routine maintenance of the instrumentation infrastructure.

Requirements:

A Bachelor's degree in an appropriate scientific field plus a minimum of ten (10) years (post-degree) of relevant and productive work experience is required OR,

A Master's degree in an appropriate scientific field plus a minimum of nine (9) years (post-degree) of relevant and productive work experience is required OR,

A PhD in an appropriate scientific field plus five (5) years (post-degree) of relevant and productive work experience is required.


To apply please visit our Web site www.stjude.org/jobs

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From: mlibbee-at-gmail.com
Date: Thu, 3 Jan 2008 13:58:10 -0600
Subject: [Microscopy] viaWWW: Denton Desk II Maintenance

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Email: mlibbee-at-gmail.com
Name: Marissa

Title-Subject: [Filtered] Denton Desk II Maintenance

Question: Greetings! I want to clean up the Denton Desk II sputter coater (equipped with AuPd target) in my lab facility. Does anyone have any suggestions as to how I to clean the plastic encasing? Are there any solvents safe to use for this purpose?

Thanks and Happy New Year!!

Marissa

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From: eschumacher-at-mccrone.com
Date: Thu, 3 Jan 2008 14:26:06 -0600
Subject: [Microscopy] Symposium: Teaching Microscopy and Microanalysis

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Greetings Colleagues,

If you are active in or interested in microscopy education, and would
like details about an M&M 08 symposium on teaching microscopy and
microanalysis, please reply offline by sending your contact information
to:

eschumacher-at-mccrone.com

We would like to compile an email address list so that we can send
information about the symposium directly to those who would like to
receive it. The symposium will cover programs for classroom teaching at
all levels, and other methods of training. Please feel free to forward
this request to interested colleagues.

Thank you,

Elaine Schumacher, McCrone Associates Charles Lyman, Lehigh
University


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From: beaurega-at-westol.com
Date: Thu, 3 Jan 2008 18:35:59 -0600
Subject: [Microscopy] Re: viaWWW: Disposable microtome blades

Contents Retrieved from Microscopy Listserver Archives
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Massimo,

Based on your words "disposable" and 'blade', I think you should try
disposable Weck Prep Extra Long Blades (2.25 inches long). These are
available from various EM supply houses in the US and maybe elsewhere.
They do say Weck on them. So check and see if that name is on one side of
the blade you got from histology. Some biologists call them surgical
blades. So check with your friend to see if that is what he gave you.

In any case, these are single edged "razor blades" designed for surgical
cutting or chopping of tissue. Weck Blades are much sharper than regular
"razor blades". In my opinion, they are about 3-5 times sharper than
ordinary razor blades based on my experience using them to block trim hard
Epon epoxy.

Once you start using them, you will stop using regular razor blades and
ignore the extra cost.

HTH,

Paul.

At 09:03 AM 1/3/08 -0600, you wrote:
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From: edelmare-at-muohio.edu
Date: Fri, 4 Jan 2008 11:57:17 -0600
Subject: [Microscopy] Re: viaWWW: Denton Desk II Maintenance

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Plastic encasing? Are you sure? Our Denton Desk II has a glass
cylinder, which we regualrly clean (the inside) of simply but
carefully running a new (cleaned) razor blade around. Slides on the
glass and peels of the metal. We remove the L-seals, and then we use
an ethanol soaked cotton coth to remove any remaining bits and finger
Prints. The aluminium bits we polish with a "Green-Scratchey-thing"
(3M) and more ethanol, then wiped down with toweling.

The only "Plastic" is the teflon bits inside, and again we use
ethanol and paper towels or cotton cloth to polish them up. The case
work is painted metals and we use general purpose glass/surface
cleaner on it.




On 3 Jan 2008 at 14:58, mlibbee-at-gmail.com wrote:

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}
} Title-Subject: [Filtered] Denton Desk II Maintenance
}
} Question: Greetings! I want to clean up the Denton Desk II sputter
} coater (equipped with AuPd target) in my lab facility. Does anyone
} have any suggestions as to how I to clean the plastic encasing? Are
} there any solvents safe to use for this purpose?
}
} Thanks and Happy New Year!!
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} Marissa
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Richard E. Edelmann, Ph.D.
Electron Microscopy Facility Director
364 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


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From: edelmare-at-muohio.edu
Date: Fri, 4 Jan 2008 13:39:03 -0600
Subject: [Microscopy] Re: AskAMicroscopist: EM film 5302

Contents Retrieved from Microscopy Listserver Archives
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Susan:

I have a full set of Kidak instructions for 5302. I can scan them
and send along if you would like.

Oh, here's Kodak's online:

http://www.kodak.com/US/plugins/acrobat/en/motion/products/lab/h15302.
pdf

But to answer:

Safelight: Kodak OA (greenish Yellow) or 1A (the deep dark red
mentioned by Patricia Stranen Connelly).

develop:

20C

Dektol (1part dektol : 2 parts water) 2 to 4 mins.

Rinse (water or stopbath)

Fix Kodak fixer 2 to 4 mins

Wash 15 to 20 mins in water or (Hypoclear 1-2 mins then 5 min wash).

I used to regularly use this film for making black and white slides
by contact printing B&W Negs. I have never used it for direct EM
Exposure. But as far as I know it is NOT a directly invertable film
(i.e. it will not give you a positive image after exposing it
directly to the beam.) It is not a "35mm slide" type of film (without
some fancy developing techniques).





On 3 Jan 2008 at 10:06, susan.trant-at-viha.ca wrote:

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} This Question was submitted to Ask-A-Microscopist by (susan.trant-at-viha.ca)
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} Email: susan.trant-at-viha.ca
} Name: Susan Trant
}
} Education: Graduate College
}
} Location: Victoria, British Columbia, Canada
}
} Title: EM film
}
} Question: Hello everyone
}
} I purchased Eastman Fine Grain Release Positive Film 5302 from
} Electron Microscopy Sciences for my TEM. The film is much thicker
} than the current product that I am using. I contacted some photo
} experts and they said that I needed a product called Dektol for a film
} developer.(Kodak) Does anyone use this film and if so, what developer
} do you use and what temperature and length of time for processing? The
} photography shop that I talked to also said that you do not dilute the
} stock solution before use. We are receiving a new digital imaging
} system within the year.
}
} Thanks
}
} Sue Trant
} EM Technologist
} Vancouver Island Health Authority
} Victoria, British Columbia,
} Canada
}
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Richard E. Edelmann, Ph.D.
Electron Microscopy Facility Director
364 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


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From: kraftpiano-at-gmail.com
Date: Fri, 4 Jan 2008 14:49:58 -0600
Subject: [Microscopy] ISI Mini-SEM

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Ok. Before you say that I'm glutton for punishment, just remember
that I really love playing with these kinds of toys...

I just picked up an ISI Mini-SEM, and got it home to play with. It
looked simple enough that I could start breaking apart the systems of
the SEM and analyzing them independently. I've got the main blue
control box with two modules in it, a brown box with what I assume is
the HV system, the chamber and column assembly (This is the smallest
chamber I've ever seen!), and the tan voltage converter box. Is there
one more piece somewhere that I should have? Does anybody have any
documentation on one of these that they could copy a page or two for
me?

Thanks,

Justin A. Kraft

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From: paul_hazelton-at-umanitoba.ca
Date: Fri, 4 Jan 2008 15:32:54 -0600
Subject: [Microscopy] Re: AskAMicroscopist: EM film 5302

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Sue

Unlike Pat, I'm still using 5302. And unlike edelmare (sorry, seen your
postings but we've never met and I don't know your name) I have always
used it for EM. Did try to use it as fine grain film for pictures of
gels many years ago, but when a 1 min exposure at F1.8 did not give
sufficient exposure I gave that up. First, you are right, the base is
more thick than the estar bases you are familiar with. I assume you
have the sprocket film - Kodak stopped producing the sproketless some
years ago. The problem with the sprocketless film was that apparently
during the cutting process the film was friction fed. As a result you
got an occasional scratch due to a piece of dust getting in the system
between the gel and a roller. Scratches tended to be quite long, and
gave the idea of 35mm film a bad name. There are essentially no
problems with scratches on the sprocket film. The thicker base makes it
also work better when loading and putting into developer spools - there
is less chance of breaking the film at the sprocket hole. This means
the Paterson steel spools work well.

As Pat said, the green/yellow OA filter is suffcient. Leaves plenty of
light to work with in the dark room.

As far as developer - we have alwoays used the D-19 developer, full
strength. Get packages to make 1G US and put into a collapsable bag -
say the type juice concentrates come in for wine making kits. This
reduces air head room and prevents oxidation of the developer. It will
keep a lot longer that way. I'm not sure about the current status for
getting developer from Kodak Canada. The last order we placed took some
time. I have the recipe for making it from scratch and can send it to
you next week if you need. On break for the rest of the week and not
back in the lab until Monday.

I under-expose slightly and push develop. The time is 3:30 at 20-22C.
If compulsive you wash with a week acetic acid stop solution (1% of
stock, or about 0.4% true concentration acetic acid). Then into any
clearing bath for 5 minutes.

The film has really fine grain. I regularly enlarge 10x for working
prints and make publication prints at 4-5 times enlargement. You will
be quite happy with the results once you get the exposure times worked out.

Since you are doing film, what chemistry are you using for your printing?

Also, Tina - if you see this - sorry about the Sugar Bowl, but if I'b
been in New Orleans, the Rainbow Warriors would have been worth the
price of admission alone.

And regards the World Under 20's in Pardubice - for the rest of you guys
on the wrong side of the 49th - final score Canada 4, US 1

Go Canada Go.

Paul

Paul R. Hazelton, PhD
Electron Microscope Unit
University of Manitoba
Department of Medical Microbiology
531 Basic Medical Sciences Building
730 William Avenue
Winnipeg, Manitoba, Canada, R3E 0W3
e-mail: paul_hazelton-at-umanitoba.ca
Phone:204-789-3313
Cell:204-781-6982
Fax:204-789- 3926


==============================Original Headers==============================
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From: mmiralles-at-pi.ac.ae
Date: Sat, 5 Jan 2008 03:18:23 -0600
Subject: [Microscopy] Training Course on ESEM

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html


Dear All,

Can anybody suggest a good training course for somebody who's new to
application of SEM/ESEM to geology?
A website link is highly appreciated.

Thank you so much.

Melina Miralles
PGSc Lab Technician
The Petroleum Institute
Abu Dhabi, UAE


==============================Original Headers==============================
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From: zaluzec-at-microscopy.com
Date: Sat, 5 Jan 2008 09:48:15 -0600
Subject: [Microscopy] Re: Training Course on ESEM

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Melina

There will be a PreMeeting Workshop covering ESEM at the
ACMM-20 Meeting in Perth Western Australia in Feb. 2008.

Here is the meeting URL : http://www.microscopy.org.au/ACMM20

Follow the link to Workshops.

Nestor
Your Friendly Neighborhood SysOp





} ----------------------------------------------------------------------------
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of America


==============================Original Headers==============================
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From: zaluzec-at-microscopy.com
Date: Sat, 5 Jan 2008 10:03:09 -0600
Subject: [Microscopy] Administrivia: 2007 Listserver Archives on-line

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Happy New Year Colleagues...

and welcome to the 15th year of operation of the Microscopy Listserver.

The archives and search engine for all of 2007 are now on-line at

http://www.microscopy.com

Nestor
Your Friendly Neighborhood SysOp



==============================Original Headers==============================
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From: Andrew.Bowling-at-ARS.USDA.GOV
Date: Sat, 5 Jan 2008 13:12:20 -0600
Subject: [Microscopy] Re: Embedding pine needles in JB-4

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Sal,

1.) I would definitely switch to LR white. We never use methacrylate
resins anymore.

2.) The flat-bottomed capsules recommended by Tobias are much better for
polymerizing LR white than BEEM-type capsules. The walls seem to be
thicker and are therefore less permeable to oxygen. Also, they are
offered in polypropylene. The PP capsules are really a pain to get the
blocks out of, but they polymerize really nicely.

3.) I was told that putting LR white (and maybe methacrylate?) resins
under vacuum can cause the initiator to evaporate from the resin,
causing incomplete polymerization. If you need to vacuum to remove air
from your needles, I would do it during fixation or during the
post-fixation wash. If you want further details, just email me.

Have fun,

Andy Bowling


-----Original Message-----
X-from: baskin-at-bio.umass.edu [mailto:baskin-at-bio.umass.edu]
Sent: Wednesday, January 02, 2008 3:50 PM
To: Bowling, Andrew

Sau,
Not sure exactly if this will solve your problem, but for what
its worth, you can get capsules that are like BEEMs except that they
have a completely flat bottom. They are made by TAAB but available from
major supply houses (no finanical connection). This gives a nice 7 mm
(or so) flat surface. You can also get this out of a standard BEEM by
flipping it upside down, although you have to mess about to keep the
resin from leaking (definitely a mess, but possible to do).

Hope this helps,
Tobias

}
} Hi,
}
} Happy New Year!!
}
} Has anyone embedded pine needles in JB-4 and sectioned for LM? I had
} problem with orientation when I used plastic beem capsules before. I
} have been trying silicon rubber molds under 10psi. But it doesn't
} polymerize competely. What is the max psi i can go not to damage both
} tissue and plastic.
} I have been also thinking of switching to LR-white.
} But I dont know if i get better result. I would appreciate any kind of
} advice on this.
}
} Thanks.
}
} Sau Silwal
}

--
_ ____ __ ____
/ \ / / \ / \ \ Tobias I. Baskin
/ / / / \ \ \ Biology Department
/_ / __ /__ \ \ \__ 611 N. Pleasant St.
/ / / \ \ \ University of
Massachusetts
/ / / \ \ \ Amherst, MA, 01003
/ / ___ / \ \__/ \ ____
http://www.bio.umass.edu/biology/baskin/
Voice: 413 - 545 - 1533 Fax: 413 - 545 - 3243

==============================Original
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From: PhillipsT-at-missouri.edu
Date: Sat, 5 Jan 2008 13:29:37 -0600
Subject: [Microscopy] Re: Embedding pine needles in JB-4

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Some methycrylates have significant advantages over LR White. We
routinely use a mixture of butyl and methylmethacrylate (BMMA) that we
got from a paper by Tobias Baskin. This resin can be removed from
sections using acetone in a manner analogous to xylene treatment of
paraffin sections. This greatly increases immunostaining. Unlike JB-4,
this resin easily cuts on water filled troughs. Since it is made from
generic methacrylate resins, it is less expensive than the proprietary
formulations. It is no good for TEM but you can't have everything. For
TEM immunocytochemistry, I prefer LR Gold to LR White since I feel it
cuts better with similar immunoreactivity.



-----Original Message-----
X-from: Andrew.Bowling-at-ARS.USDA.GOV [mailto:Andrew.Bowling-at-ARS.USDA.GOV]
Sent: Saturday, January 05, 2008 1:14 PM
To: Phillips, Thomas E.

Sal,

1.) I would definitely switch to LR white. We never use methacrylate
resins anymore.

2.) The flat-bottomed capsules recommended by Tobias are much better for
polymerizing LR white than BEEM-type capsules. The walls seem to be
thicker and are therefore less permeable to oxygen. Also, they are
offered in polypropylene. The PP capsules are really a pain to get the
blocks out of, but they polymerize really nicely.

3.) I was told that putting LR white (and maybe methacrylate?) resins
under vacuum can cause the initiator to evaporate from the resin,
causing incomplete polymerization. If you need to vacuum to remove air
from your needles, I would do it during fixation or during the
post-fixation wash. If you want further details, just email me.

Have fun,

Andy Bowling


-----Original Message-----
X-from: baskin-at-bio.umass.edu [mailto:baskin-at-bio.umass.edu]
Sent: Wednesday, January 02, 2008 3:50 PM
To: Bowling, Andrew

Sau,
Not sure exactly if this will solve your problem, but for what
its worth, you can get capsules that are like BEEMs except that they
have a completely flat bottom. They are made by TAAB but available from
major supply houses (no finanical connection). This gives a nice 7 mm
(or so) flat surface. You can also get this out of a standard BEEM by
flipping it upside down, although you have to mess about to keep the
resin from leaking (definitely a mess, but possible to do).

Hope this helps,
Tobias

}
} Hi,
}
} Happy New Year!!
}
} Has anyone embedded pine needles in JB-4 and sectioned for LM? I had
} problem with orientation when I used plastic beem capsules before. I
} have been trying silicon rubber molds under 10psi. But it doesn't
} polymerize competely. What is the max psi i can go not to damage both
} tissue and plastic.
} I have been also thinking of switching to LR-white.
} But I dont know if i get better result. I would appreciate any kind of
} advice on this.
}
} Thanks.
}
} Sau Silwal
}

--
_ ____ __ ____
/ \ / / \ / \ \ Tobias I. Baskin
/ / / / \ \ \ Biology Department
/_ / __ /__ \ \ \__ 611 N. Pleasant St.
/ / / \ \ \ University of
Massachusetts
/ / / \ \ \ Amherst, MA, 01003
/ / ___ / \ \__/ \ ____
http://www.bio.umass.edu/biology/baskin/
Voice: 413 - 545 - 1533 Fax: 413 - 545 - 3243

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26, 25 -- From PhillipsT-at-missouri.edu Sat Jan 5 13:29:37 2008
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From: kenconverse-at-qualityimages.biz
Date: Sat, 5 Jan 2008 19:28:33 -0600
Subject: [Microscopy] Re: viaWWW: Denton Desk II Maintenance

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Marissa,
If it turns out that your chamber is glass (which I suspect), after you get
it clean, buy yourself a can of unscented White Rain hairspray and spray the
inside surface of the glass tube (I would hesitate to do this to plastic
because of the possibility of incompatible solvents). The next time you
want to clean, just place the glass in hot soapy water. When the hairspray
dissolves, your Au/Pd will also depart with little or no effort, and no
scratches or cut fingers.

Ken Converse
owner

QUALITY IMAGES
Servicing Scanning Electron Microscopes
Since 1981
474 So. Bridgton Rd.
Bridgton, ME 04009
207-647-4348
Fax 207-647-2688
kenconverse-at-qualityimages.biz
qualityimages.biz



-----Original Message-----
X-from: edelmare-at-muohio.edu [mailto:edelmare-at-muohio.edu]
Sent: Friday, January 04, 2008 1:02 PM
To: kenconverse-at-qualityimages.biz

Plastic encasing? Are you sure? Our Denton Desk II has a glass
cylinder, which we regualrly clean (the inside) of simply but
carefully running a new (cleaned) razor blade around. Slides on the
glass and peels of the metal. We remove the L-seals, and then we use
an ethanol soaked cotton coth to remove any remaining bits and finger
Prints. The aluminium bits we polish with a "Green-Scratchey-thing"
(3M) and more ethanol, then wiped down with toweling.

The only "Plastic" is the teflon bits inside, and again we use
ethanol and paper towels or cotton cloth to polish them up. The case
work is painted metals and we use general purpose glass/surface
cleaner on it.




On 3 Jan 2008 at 14:58, mlibbee-at-gmail.com wrote:

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} Email: mlibbee-at-gmail.com
} Name: Marissa
}
} Title-Subject: [Filtered] Denton Desk II Maintenance
}
} Question: Greetings! I want to clean up the Denton Desk II sputter
} coater (equipped with AuPd target) in my lab facility. Does anyone
} have any suggestions as to how I to clean the plastic encasing? Are
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} 7, 11 -- From zaluzec-at-microscopy.com Thu Jan 3 13:58:09 2008
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Richard E. Edelmann, Ph.D.
Electron Microscopy Facility Director
364 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


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From: dhitrys-at-qimaging.com
Date: Sun, 6 Jan 2008 16:30:47 -0600
Subject: [Microscopy] This week's microscopy webinar schedule

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

You are invited to attend our upcoming live, interactive, web-based
instructional microscopy seminars.

Pre-registration is required and connection lines are limited so reserve
yours now. There is no charge to participate.

See further descriptions and pre-register at:
http://www.magbiosystems.com/education


Coming up this week (January 7 - 11):

==========================================================
"Quantitative Image and Data Acquisition for Fluorescent Specimens"
Advice from a Facility Director

Presented by Brian Matsumoto, Ph.D., University of California, Santa Barbara

Monday, 07-January at 1:30 PM (New York time)

==========================================================
"Live Cell Fluorescent Imaging"

Presented by Nicholas Beavers, Media Cybernetics

Wednesday, 09-January at 1:30 PM (New York time)

==========================================================
"Tracking Objects in 2D and 3D"

Presented by Paul Jantzen, Media Cybernetics

Friday, 11-January at 1:30 PM (New York time)

==========================================================

Calendar, descriptions, and pre-registration is at:
http://www.magbiosystems.com/education


Seminars require that attendees use a Java-enabled browser with a high
bandwidth connection. Audio is via toll-free telephone.

==============================Original Headers==============================
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From: gary.m.brown-at-exxonmobil.com
Date: Mon, 7 Jan 2008 13:51:21 -0600
Subject: [Microscopy] Re: viaWWW: Image processing software

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Rao,

I recommend Adobe Photoshop with plug-in Image Processing Tool Kit or
FoveaPro, both from Reindeer Graphics for your image analysis needs.

Regards,

Gary M. Brown
Microscopy Specialist
ExxonMobil Chemical Company
Baytown Technology & Engineering - West
5200 Bayway Drive
Baytown, Texas 77520-2101
phone: 281 834 2387
fax: 281 834 2395
e-mail: Gary.M.Brown-at-ExxonMobil.com

"Our business in life is not to succeed, but to continue to fail in good
spirits." Robert Louis Stevenson






rao5-at-hotmail.c
om
To
gary.m.brown-at-exxonmobil.com
12/26/07 09:14 cc
AM
Subject
[Microscopy] viaWWW: Image
Please respond processing software
to
rao5-at-hotmail.c
om











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Email: rao5-at-hotmail.com
Name: Venkat Bommisetty

Organization: SDSU

Title-Subject: [Filtered] Image processing software

Question: Hi All,
Greetings for Merry X-mas and New Year....
Is there any general purpose image processing software that can do grain
size analysis? I like to process AFM, SEM and TEM images eithr in their
native format or as bitmaps.

Also, do you recommend any software for processing Selective area
diffraction patterns? currently I write IDL code again, not very easy for
students to use.

In both cases the software is intended to be used for use in teaching &
research both. Price is an important concern


thanks in advance for your advice

Rao

Login Host: 12.201.57.158
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From: pmccurdy-at-lamar.colostate.edu
Date: Mon, 7 Jan 2008 15:52:43 -0600
Subject: [Microscopy] AskAMicroscopist: Cleaning a Moly aperture

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Email: pmccurdy-at-lamar.colostate.edu
Name: Pat McCurdy

Organization: Colorado State University

Education: Graduate College

Location: Fort Collins, Colorado, USA

Title: Cleaning a Moly aperture

Question: Is it possible to use an argon ion gun to clean a moly SEM aperture? If not, why not?

Thanks,
Pat McCurdy
Colorado State University

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From: andrea-at-ncmir.ucsd.edu
Date: Mon, 7 Jan 2008 15:53:39 -0600
Subject: [Microscopy] viaWWW: problems cutting serial thick sections (above 1-2

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Email: andrea-at-ncmir.ucsd.edu
Name: Andrea Thor

Organization: UCSD

Title-Subject: [Filtered] problems cutting serial thick sections (above 1-2 microns) without getting serious pitting of the blockface

Question: I am having some problems in cutting serial thick sections (above 1-2 microns) without getting serious pitting of the blockface. I heard this is not uncommon when pushing the section thickness to the extreme (such as 3-5 microns). We usually deal with the situation by refacing the block after each thick section, but this of course would make true "serial" sectioning impossible.
The blocks I am working with are either cardic left ventricle or striatal tissue embedded in Durcupan.


If anyone has tried or has a protocol or techniques,
I'd be very grateful to hear about them. It
could save us tons of time and frustration as we develop a new set of protocols.

Thanks very much.

Andrea


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11, 12 -- microns) without getting serious pitting of the blockface
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From: levilr-at-hughes.net
Date: Mon, 7 Jan 2008 15:54:25 -0600
Subject: [Microscopy] viaWWW: Goniometer eyepiece

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Email: levilr-at-hughes.net
Name: Lee Levine

Organization: Consultant

Title-Subject: [Filtered] Goniometer eyepiece

Question: I saw a simple goniometer eyepiece for measuring contact angle. Does anyone know who sells these?

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From: dean-abel-at-uiowa.edu
Date: Mon, 7 Jan 2008 16:51:32 -0600
Subject: [Microscopy] Re: : problems cutting serial thick sections

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hello Andrea,
What kind of knife are you using? I get good results cutting
serial thick sections of resin embedded tissues from 1 to 5 microns
with a Diatome Diamond Histo-Knife. I have never experienced
"pitting" of the block face. I have my own bag of tricks for
collecting sections as they sometimes curl up like a wood shaving as
they come off the knife especially the thicker ones.
Dean Abel
Biological Sciences
University of Iowa
Iowa City IA 52242

At 03:56 PM 1/7/2008, you wrote:

} Email: andrea-at-ncmir.ucsd.edu
} Name: Andrea Thor
} Organization: UCSD
}
} Title-Subject: problems cutting serial thick sections (above 1-2
} microns) without getting serious pitting of the blockface
}
} Question: I am having some problems in cutting serial thick sections
} (above 1-2 microns) without getting serious pitting of the
} blockface. I heard this is not uncommon when pushing the section
} thickness to the extreme (such as 3-5 microns). We usually deal
} with the situation by refacing the block after each thick section,
} but this of course would make true "serial" sectioning impossible.
} The blocks I am working with are either cardic left ventricle or
} striatal tissue embedded in Durcupan.
}
} If anyone has tried or has a protocol or techniques, I'd be very
} grateful to hear about them. It could save us tons of time and
} frustration as we develop a new set of protocols. Thanks very much.
}
} Andrea



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5, 22 -- Microscopy Society of America
5, 22 -- {Microscopy-at-msa.microscopy.com}
5, 22 -- From: Dean Abel {dean-abel-at-uiowa.edu}
5, 22 -- Subject: Re: [Microscopy]: problems cutting serial thick sections
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From: FChu-at-mrl.ubc.ca
Date: Mon, 7 Jan 2008 17:34:00 -0600
Subject: [Microscopy] Adhesive for methyl methacrylate (Technovit 9100 Embedding

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Instead of using "Technovit 3040", I am looking for an alternative glue
for methyl methacrylate (Technovit 9100 Embedding Medium).

Any suggestions would be appreciated.

What I need is:
- a mounting medium/glue/adhesive of some sort to attach metal stubs to
specimen which have been embedded in methyl methacrylate (Technovit 9100
Embedding Medium).

The company has suggested Technovit* 3040 which:
(1) is a yellow, fast-curing (5-10 minutes, depending on room
temperature) methyl methacrylate-based resin.

(2) has a "chemical composition that warrants a firm, durable bond with
Technovit and secure fixing of the specimens to the Histobloc."

(3) consists of "two components- powder and liquid- allowing simple
mixing, easy adhering to the specimen, and fast curing. For fixing the
mounts, a highly viscous consistency (i.e., a mixing ratio of
approximately 2-3 parts per volume powder: 1 part per volume liquid) has
proven to be the most advantageous."

Thanks in advance,

Fanny Chu
Ultrastructural Imaging
The James C Hogg iCAPTURE Lab,
University of British Columbia,
St. Paul's Hospital Site
Rm 166, 1081 Burrard St,
Vancouver, BC, Canada
(604) 806-8346, x62712, x62703



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From: baskin-at-bio.umass.edu
Date: Mon, 7 Jan 2008 17:44:51 -0600
Subject: [Microscopy] Re: Adhesive for methyl methacrylate (Technovit 9100 Embedding

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi,
For what its worth, I have glued methacrylate blocks
(mixtures of methyl and butyl) to epoxy stubs with cyanoacrylate type
adhesives (brand name Krazy Glue, among others). THese adhesives are
known in general to stick to metal, and they are cheap and available
at any hardware store. Might work?

In this case, I hope you *do* get stuck! 8--).

Tobias

}
}
} Instead of using "Technovit 3040", I am looking for an alternative glue
} for methyl methacrylate (Technovit 9100 Embedding Medium).
}
} Any suggestions would be appreciated.
}
} What I need is:
} - a mounting medium/glue/adhesive of some sort to attach metal stubs to
} specimen which have been embedded in methyl methacrylate (Technovit 9100
} Embedding Medium).
}
} The company has suggested Technovit* 3040 which:
} (1) is a yellow, fast-curing (5-10 minutes, depending on room
} temperature) methyl methacrylate-based resin.
}
} (2) has a "chemical composition that warrants a firm, durable bond with
} Technovit and secure fixing of the specimens to the Histobloc."
}
} (3) consists of "two components- powder and liquid- allowing simple
} mixing, easy adhering to the specimen, and fast curing. For fixing the
} mounts, a highly viscous consistency (i.e., a mixing ratio of
} approximately 2-3 parts per volume powder: 1 part per volume liquid) has
} proven to be the most advantageous."
}
} Thanks in advance,
}
} Fanny Chu
} Ultrastructural Imaging
} The James C Hogg iCAPTURE Lab,
} University of British Columbia,
} St. Paul's Hospital Site
} Rm 166, 1081 Burrard St,
} Vancouver, BC, Canada
} (604) 806-8346, x62712, x62703
}

--
_ ____ __ ____
/ \ / / \ / \ \ Tobias I. Baskin
/ / / / \ \ \ Biology Department
/_ / __ /__ \ \ \__ 611 N. Pleasant St.
/ / / \ \ \ University of Massachusetts
/ / / \ \ \ Amherst, MA, 01003
/ / ___ / \ \__/ \ ____
http://www.bio.umass.edu/biology/baskin/
Voice: 413 - 545 - 1533 Fax: 413 - 545 - 3243

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From: jmkrupp-at-ucsc.edu
Date: Mon, 7 Jan 2008 18:10:23 -0600
Subject: [Microscopy] How do you charge for use?

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi:

My bean counters are at it again. I have been asked to look into the
ways other labs charge for using equipment.

We have always charged by the hour as recorded on a meter that runs
when the filament is on. Minimum charge is 0.1 hour. No charges for
using specimen prep equipment or for my time other than the cost of
consumable supplies.

They are asking about things like minimum charges, like 1 hour
minimum to start, charging based on time and extent of 'room' use,
charging a portion of my salary in addition to filament time, etc.

It is pretty much a brainstorming activity for now, so anything goes.

Jon


--

Jonathan Krupp
Microscopy & Imaging Lab
C230 Earth & Marine Science
University of California
Santa Cruz, CA 95064
(831) 459-2477
jmkrupp-at-ucsc.edu

I rode in AIDS/Lifecycle 6 SF to LA June 3 - 9, 2007 to raise money
for the San Francisco AIDS Foundation. Visit
http://www.aidslifecycle.org for more information about the ride.

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From: dsams-at-schaferlabs.com
Date: Mon, 7 Jan 2008 18:37:27 -0600
Subject: [Microscopy] Job Posting: Mass Spectrometry Staff Engineer / Scientist

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Overview: Schafer Corporation, Sunol, CA, is seeking a skilled and
innovative Staff Engineer / Scientist to add to our mass spectrometry group.
SVL performs materials characterization and related analytical services on
commercial and government contracts. The activities of the group include
chemical and elemental analysis of materials on a production basis,
maintenance of several mass spectrometers and ancillary equipment,
development of new and improved analysis techniques, interpretation, and
quality assurance of analytical data. The successful candidate will
primarily write software, operate instruments, perform QC/QA, reduce, and
analyze data.

Responsibilities: Primary duties include scientific analytical programming,
instrument operation and maintenance, developing and optimizing analytical
techniques, statistical analysis, and data interpretation. Will prepare and
make presentations on technical findings. As a lead engineer or scientist,
this individual will be a key resource for Schafer and our customers,
maintaining our expertise in the field of high sensitivity, high precision
isotopic analysis.

Qualifications: The ideal candidate must have a strong background in
materials science or engineering, or a related field of physics, geology,
chemistry, statistics, or mathematics. Should have experience in a
scientific laboratory, preferably operating SIMS, TIMS, SEM, or TEM.
Experience with high vacuum technology, electronics, mechanical design,
cryogenic system, and ion optics is helpful. Should have demonstrated
scientific programming experience (such as Labview or FORTRAN), including
statistical analysis and data interpretation. Database familiarity is
helpful. Must be able to work independently and as part of a team of
scientists, engineers, and technicians. Good customer service focus and
commitment to quality are required.

Other qualifications include:
• Bachelor's degree in physical science or engineering with minimum 5
years of technical experience.
• Demonstrated ability to perform complex professional engineering /
scientific work, including scientific analysis, planning, and execution.
• Analytical laboratory experience in software, statistics, data
evaluation, and quality control.
• Proven ability to clearly write and present scientific reports and
proposals.
• Must be a US citizen with the ability to obtain government security
clearance.

Apply at:
http://jobs-schafer.icims.com/schafer_jobs/jobs/candidate/job.jsp?jobid=1331
&mode=view
Schafer Corporation is an Affirmative Action, Equal Opportunity Employer.

David Sams, Ph.D.
Group Leader, Mass Spectrometry
AEM Group
Schafer Laboratories
6705 Vallecitos Rd.
Sunol, CA 94586
dsams-at-schaferlabs.com



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8, 20 -- Subject: Job Posting: Mass Spectrometry Staff Engineer / Scientist
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From: Rosemary.White-at-csiro.au
Date: Mon, 7 Jan 2008 20:50:42 -0600
Subject: [Microscopy] Re: How do you charge for use?

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi Jon,

We used to do this, indeed, we were supposed to operate under "full cost
recovery". However, in their wisdom(?), the corporate types in our
organisation decided that any "unit" with operational costs (including
salaries) less than $1 million per year could stop charging like this and be
funded entirely from overheads. We still have to charge outsiders, and
still record instrument use, but no more charging. From one extreme to the
other.....

cheers,
rosemary

Rosemary White rosemary.white-at-csiro.au
CSIRO Plant Industry ph. 61 (0)2-6246 5475
GPO Box 1600 fax. 61 (0)2-6246 5334
Canberra, ACT 2601
Australia



On 8/1/08 11:15 AM, "jmkrupp-at-ucsc.edu" {jmkrupp-at-ucsc.edu} wrote:

}
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} ----------------------------------------------------------------------------
}
} Hi:
}
} My bean counters are at it again. I have been asked to look into the
} ways other labs charge for using equipment.
}
} We have always charged by the hour as recorded on a meter that runs
} when the filament is on. Minimum charge is 0.1 hour. No charges for
} using specimen prep equipment or for my time other than the cost of
} consumable supplies.
}
} They are asking about things like minimum charges, like 1 hour
} minimum to start, charging based on time and extent of 'room' use,
} charging a portion of my salary in addition to filament time, etc.
}
} It is pretty much a brainstorming activity for now, so anything goes.
}
} Jon
}


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9, 25 -- Date: Tue, 08 Jan 2008 13:54:23 +1100
9, 25 -- Subject: Re: [Microscopy] How do you charge for use?
9, 25 -- From: Rosemary White {Rosemary.White-at-csiro.au}
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From: a.d.mckinnon-at-abdn.ac.uk
Date: Tue, 8 Jan 2008 05:57:40 -0600
Subject: [Microscopy] viaWWW: problems cutting serial thick sections

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Jill

I have no experience with the Coolwell cooler that you mention but the
symptoms sound similar to our UK Flowcool cooler.

After 2 or 3 years the temperature readout becomes erratic and when I
contacted the supplier/manufacturer they told me to replace the
temperature probe in the water tank. They have supplied me with spares
and on my machine it is a relatively simple operation.

If you can still contact the manufacturer maybe they can help.

Good luck.

Malcolm

Malcolm Haswell
e.m. unit
Chemispec
School of Health, Natural and Social Sciences
Fleming Building
University of Sunderland
Tyne & Wear
SR1 3SD
UK
e-mail: malcolm.haswell-at-sunderland.ac.uk



----- Original Message -----
X-from: Jill.Verlander-at-medicine.ufl.edu

Hi Andrea,

Briefly, this type of problem is down to brittle resin blocks being
sectioned at too fast a cutting speed and the thicker the section, the
more likely it is to occur.

Try adjusting the hardener/plasticiser proportion of your embedding mix
and/or reducing the polymerisation time/temperature to end up with a
softer block.

With the blocks already processed, use the best available knife and
reduce the cutting speed. If the chipping of the face recurs, your only
remaining option is to reduce the section thickness.

Like Dean Abel suggests, I would be using a histodiamond (wet) with a
cutting window speed of 1mm/sec and increasing the section thickness
gradually from an initial 2 microns. I would also trim off most of the
surrounding resin and shape the block to a point to reduce the cutting
force on the knife, particularly as you are wanting to section at up to
5 microns.

Happy New Year!

Alastair McKinnon
Histology & EM Facility Manager
University of Aberdeen, Institute of Medical Science
Foresterhill, Aberdeen, Scotland, AB25 2ZD
tel: +44(0)1224 552923 (office); +44(0)1224 555911 (lab)
fax: +44(0)1224 559533; email: a.d.mckinnon-at-abdn.ac.uk
www.abdn.ac.uk/ims/h-em
-----Original Message-----
X-from: andrea-at-ncmir.ucsd.edu [mailto:andrea-at-ncmir.ucsd.edu]
Sent: 07 January 2008 22:02
To: Mckinnon, Alastair D.

This Question/Comment was submitted to the Microscopy Listserver using
the WWW based Form at
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Email: andrea-at-ncmir.ucsd.edu
Name: Andrea Thor

Organization: UCSD

Title-Subject: [Filtered] problems cutting serial thick sections (above
1-2 microns) without getting serious pitting of the blockface

Question: I am having some problems in cutting serial thick sections
(above 1-2 microns) without getting serious pitting of the blockface. I
heard this is not uncommon when pushing the section thickness to the
extreme (such as 3-5 microns). We usually deal with the situation by
refacing the block after each thick section, but this of course would
make true "serial" sectioning impossible.
The blocks I am working with are either cardic left ventricle or
striatal tissue embedded in Durcupan.


If anyone has tried or has a protocol or techniques, I'd be very
grateful to hear about them. It could save us tons of time and
frustration as we develop a new set of protocols.

Thanks very much.

Andrea


Login Host: 132.239.22.218
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From: PetrS-at-ISIBrno.Cz
Date: Wed, 9 Jan 2008 08:39:47 -0600
Subject: [Microscopy] Meetings for Microscopists in 2008

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi Jon,
We charge per/hour for equipment use: TEM, SEM, CPD, Sputter Coater, Digital
LM and any dark room use (yes there are still a couple of researches using
film!!).We do not allow users to process their samples here as there is not
enough room nor do we train them. We can process the tissue for them at a
price per every 2 samples (we figure an experimental and a control is pretty
standard). This processing charge includes supplies and our time. We then
charge per block for thick sections and another charge for thin sectioning.
Our time is charged at rates that take into consideration who's hands are
helping/training: SRA I, SRAII or SRAIV. We do have a few supplies we will
sell to the researcher at our cost (tax and shipping figured into the
equation): stubs, coated grids, 16% paraformaldehyde, etc.
Hope this helps!
Pat Kysar
University of California, Davis
Medical School, Pathology
EM Lab
530-752-4701

----- Original Message -----
X-from: {jmkrupp-at-ucsc.edu}
To: {pekysar-at-ucdavis.edu}
Sent: Monday, January 07, 2008 4:15 PM

Dear Microscopists,

The first update of the list of meetings for microscopists in the year
2008 has been finished at the Petr's Microscopy Resources at the

http://www.petr.isibrno.cz/microscopy/meetings.php#2008

Your submission of other meetings will be very appreciated (submission
form is accessible from the page mentioned, the direct link for the
submission is http://www.petr.isibrno.cz/microscopy/PMRform.php).

Regards,
Petr Schauer
********************************************
Dr. Petr Schauer
Scintillation and Cathodoluminescent Systems
Institute of Scientific Instruments, AS CR, v.v.i.
Academy of Sciences of the Czech Republic
Kralovopolska 147, CZ-61264 Brno, Czech Republic
********************************************
tel.: +420 541 514 313
fax : +420 541 514 404, or +420 541 514 402
e-mail: petr-at-isibrno.cz
www: http://www.petr.isibrno.cz/
********************************************


==============================Original Headers==============================
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From: hkonishi-at-wisc.edu
Date: Wed, 9 Jan 2008 09:24:37 -0600
Subject: [Microscopy] Thermo/Noran EDS: How to convert eds to emsa file?

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hello:

I am looking for a free software to convert eds to emsa extension file.

I am using an old software for Thermo/Noran EDS. It has two types of
file format: Vantage (eds extension) and EMSA (emsa extension). Recent
NORAN System Six can read emsa format, but not eds format.

I can open eds file using old software and save as emsa format.
However, it is inconvenient. Is there any alternative method (like
free software) to convert eds format to emsa format? Please advise.

Thank you,

Hiromi Konishi, Ph.D.
UW-MADISON

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From: bbandli-at-mvainc.com
Date: Wed, 9 Jan 2008 09:59:26 -0600
Subject: [Microscopy] Re: Thermo/Noran EDS: How to convert eds to emsa file?

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hiromi,
Speak with your Thermo service folks. There is a software application
they have that converts .eds format (and all the other Vantage file
formats .grey etc.) to formats that are compatible with the System SIX
software. It is intended as a one-time only tool to be used during the
upgrade from a Vantage system to a System SIX system, but if you speak
with their technical service folks, they might be able to work out a
solution for you.

Good Luck,
Bryan Bandli

hkonishi-at-wisc.edu wrote:
} ----------------------------------------------------------------------------
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} Hello:
}
} I am looking for a free software to convert eds to emsa extension file.
}
} I am using an old software for Thermo/Noran EDS. It has two types of
} file format: Vantage (eds extension) and EMSA (emsa extension). Recent
} NORAN System Six can read emsa format, but not eds format.
}
} I can open eds file using old software and save as emsa format.
} However, it is inconvenient. Is there any alternative method (like
} free software) to convert eds format to emsa format? Please advise.
}
} Thank you,
}
} Hiromi Konishi, Ph.D.
} UW-MADISON
}
} ==============================Original Headers==============================
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--
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From: corrie.van-hoek-at-corusgroup.com
Date: Thu, 10 Jan 2008 04:42:41 -0600
Subject: [Microscopy] EBSD: CSL numberfractions

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html



Hi EBSD-users,

Is there some one who knows how to calculate  number fractions (not length
or pixellength fractions) of CSL boundaries (or grainboundaries in general)
from TSL and / or HKL Channel Five datasets?

Thanks for thinking along with me,


Corrie
-----------------------------------------------------------
Corrie van Hoek

CORUS RD & T
Ceramics Research Center
Building Code 3J-22
PO Box 1000
1970 CA Ijmuiden
The Netherlands
tel. 02514 92626    fax. 02514 70489

**********************************************************************
This transmission is confidential and must not be used or disclosed by
anyone other than the intended recipient. Neither Corus Group Limited nor
any of its subsidiaries can accept any responsibility for any use or
misuse of the transmission by anyone.

For address and company registration details of certain entities
within the Corus group of companies, please visit
http://www.corusgroup.com/entities

**********************************************************************



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From: nizets2-at-yahoo.com
Date: Thu, 10 Jan 2008 06:40:52 -0600
Subject: [Microscopy] Product for watercooling

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi!
During some works in a room next to our TEM, one worker opened a canalisation of the watercooling system, emptying the water tank of the watercooling device.
I filled it again with normal tap water but I think I have to add some product to avoid mold growth.
Could you recommend one such product and where I can order it, especially those of you from Germany and Austria (we are located in Vienna, Austria)?
Our microscope is a Tecnai G20 and the watercooling unit is a Zephy ZEM 1000S.

Thank you in advance,
Stephane


____________________________________________________________________________________
Never miss a thing. Make Yahoo your home page.
http://www.yahoo.com/r/hs

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From: allan.mitchell-at-stonebow.otago.ac.nz
Date: Thu, 10 Jan 2008 16:44:06 -0600
Subject: [Microscopy] Bal-Tec 060 Freeze Etching System

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi all, happy new year all

We have just inherited a BAL-TEC 060 freeze fracture system.

I would like to ask if anyone out in there Microscopy Land has
similar equipment and has written their own set of operation notes
for this system that they would be willing to share with us, perhaps
as a pdf file or similar?

We have also inherited with the freeze fracture system a Bal-Tec SBU
020 sandblasting Unit. Does anyone have one of these also and be
wiling to share the operating notes?

Many thanks, kind regards

Allan



Allan Mitchell
Technical Manager
Otago Centre for Electron Microscopy
Department of Anatomy and Structural Biology
School of Medical Sciences
P.O. Box 913
Dunedin
New Zealand

Phone (03) 479 5642 or 479 7301
Fax (03) 479 5086 or 479 7254



==============================Original Headers==============================
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From: gary-at-gaugler.com
Date: Thu, 10 Jan 2008 16:56:56 -0600
Subject: [Microscopy] Re: Product for watercooling

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

I would suggest draining the water and replacing with
distilled water. The Cl in tap water could lead to
corrosion of metal in contact with the water. A good
additive IMO is Ethylene Glycol as a 10% mix. I use
technical grade EG and add 1/2 gallon to the 4.5 gallons
of distilled water for 5 gallons total in the Haskris
R050 chiller reservoir.

Sometimes this holds up for a year.

gary g.



At 04:52 AM 1/10/2008, you wrote:




} ----------------------------------------------------------------------------
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==============================Original Headers==============================
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11, 20 -- From: Gary Gaugler {gary-at-gaugler.com}
11, 20 -- Subject: Re: [Microscopy] Product for watercooling
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From: donovan-at-uoregon.edu
Date: Fri, 11 Jan 2008 10:37:25 -0600
Subject: [Microscopy] Re: Product for watercooling

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi,

We incorporate Sigma water bath treatment in the reservoir - 3.5ml per
tank full (25L).

Seems to work well - lasting about 12 months and got this recommendation
from Sigma Technical Services re using it in chiller circulators for
EMs.

TechServ_Number: S5525
TechServ_Name: SigmaClean; water bath treatment
TechServ_Brand: SIGMA

TechServ_re: is this product recommended for use in chiller circulators
for
the supply of cooling water for a transmission EM (Philips CM10).

Best regards,

Alastair

Alastair McKinnon
Histology & EM Facility Manager, IMS R2.62
University of Aberdeen, Institute of Medical Science
Foresterhill, Aberdeen, AB25 2ZD
tel: +44(0)1224 552923 (office); +44(0)1224 555911 (lab)
fax: +44(0)1224 559533; email: a.d.mckinnon-at-abdn.ac.uk
www.abdn.ac.uk/ims/h-em
-----Original Message-----
X-from: gary-at-gaugler.com [mailto:gary-at-gaugler.com]
Sent: 10 January 2008 23:00
To: Mckinnon, Alastair D.

I would suggest draining the water and replacing with distilled water.
The Cl in tap water could lead to corrosion of metal in contact with the
water. A good additive IMO is Ethylene Glycol as a 10% mix. I use
technical grade EG and add 1/2 gallon to the 4.5 gallons of distilled
water for 5 gallons total in the Haskris R050 chiller reservoir.

Sometimes this holds up for a year.

gary g.



At 04:52 AM 1/10/2008, you wrote:




} -----------------------------------------------------------------------
} ----- The Microscopy ListServer -- CoSponsor: The Microscopy Society
} of America To Subscribe/Unsubscribe --
} http://www.microscopy.com/MicroscopyListserver

} watercooling device.
} I filled it again with normal tap water but I think I have to add some
} product to avoid mold growth.
} Could you recommend one such product and where I can order it,
} especially those of you from Germany and Austria (we are located in
} Vienna, Austria)?
} Our microscope is a Tecnai G20 and the watercooling unit is a Zephy ZEM
1000S.
}
} Thank you in advance,
} Stephane


==============================Original
Headers==============================
11, 20 -- From gary-at-gaugler.com Thu Jan 10 16:56:56 2008 11, 20 --
Received: from qsmtp4.mc.surewest.net (qsmtp.mc.surewest.net
[66.60.130.145])
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16:56:56 -0600
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All,
After much fighting of corrosion and algae issues I settled years ago
on what might be the easiest and most long term "solution". That is
pure distilled water. And here's the secret, you don't need to add
any chemical additives if you remove all clear plastic hoses from the
system and replace them with black or otherwise opaque materials. No
light, no growth.

With this "solution" I have found I can run for years with a crystal
clear tank and with only an occasional speck of rust visible in the
bottom of the tank, which is probably left over from the prior years
of running god know what through the lines. This "solution" is
currently running in several SEMs and microprobes, using a variety of
chillers (mostly Haskris which I have found to be much more reliable
than Coolwell).

Works for me anyway.
john

At 07:58 AM 1/11/2008, a.d.mckinnon-at-abdn.ac.uk wrote:



} ----------------------------------------------------------------------------
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of America


==============================Original Headers==============================
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From: bbandli-at-mvainc.com
Date: Fri, 11 Jan 2008 10:56:18 -0600
Subject: [Microscopy] Re: Product for watercooling

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

I second John's "solution". It's what we have been using for our FESEM
for several years without any problems. Opaque lines from the chiller
to the scope are essential however. Even though this is what this scope
has been on since day 1, we do have a small amount of rust/grit in the
bottom of the tank but it hasn't been a problem. We also change the H2O
every 6months (Per JEOL service).
Cheers,
Bryan Bandli

donovan-at-uoregon.edu wrote:
} ----------------------------------------------------------------------------
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of America
} To Subscribe/Unsubscribe -- http://www.microscopy.com/MicroscopyListserver
} On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} ----------------------------------------------------------------------------
}
} All,
} After much fighting of corrosion and algae issues I settled years ago
} on what might be the easiest and most long term "solution". That is
} pure distilled water. And here's the secret, you don't need to add
} any chemical additives if you remove all clear plastic hoses from the
} system and replace them with black or otherwise opaque materials. No
} light, no growth.
}
} With this "solution" I have found I can run for years with a crystal
} clear tank and with only an occasional speck of rust visible in the
} bottom of the tank, which is probably left over from the prior years
} of running god know what through the lines. This "solution" is
} currently running in several SEMs and microprobes, using a variety of
} chillers (mostly Haskris which I have found to be much more reliable
} than Coolwell).
}
} Works for me anyway.
} john
}
} At 07:58 AM 1/11/2008, a.d.mckinnon-at-abdn.ac.uk wrote:
}
}
}
}
} } ----------------------------------------------------------------------------
} } The Microscopy ListServer -- CoSponsor: The Microscopy Society of America
} } To Subscribe/Unsubscribe -- http://www.microscopy.com/MicroscopyListserver
} } On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} } ----------------------------------------------------------------------------
} }
} } Hi,
} }
} } We incorporate Sigma water bath treatment in the reservoir - 3.5ml per
} } tank full (25L).
} }
} } Seems to work well - lasting about 12 months and got this recommendation
} }
} } from Sigma Technical Services re using it in chiller circulators for
}
} } EMs.
} }
} } TechServ_Number: S5525
} } TechServ_Name: SigmaClean; water bath treatment
} } TechServ_Brand: SIGMA
} }
} } TechServ_re: is this product recommended for use in chiller circulators
} } for
} } the supply of cooling water for a transmission EM (Philips CM10).
} }
} } Best regards,
} }
} } Alastair
} }
} } Alastair McKinnon
} } Histology & EM Facility Manager, IMS R2.62
} } University of Aberdeen, Institute of Medical Science
} } Foresterhill, Aberdeen, AB25 2ZD
} } tel: +44(0)1224 552923 (office); +44(0)1224 555911 (lab)
} } fax: +44(0)1224 559533; email: a.d.mckinnon-at-abdn.ac.uk
} } www.abdn.ac.uk/ims/h-em
} } -----Original Message-----
} } X-from: gary-at-gaugler.com [mailto:gary-at-gaugler.com]
} } Sent: 10 January 2008 23:00
} } To: Mckinnon, Alastair D.
} } Subject: [Microscopy] Re: Product for watercooling
} }
} }
} }
} }
} } ------------------------------------------------------------------------
} } ----
} } The Microscopy ListServer -- CoSponsor: The Microscopy Society of
} } America To Subscribe/Unsubscribe --
} } http://www.microscopy.com/MicroscopyListserver
} } On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} } ------------------------------------------------------------------------
} } ----
} }
} } I would suggest draining the water and replacing with distilled water.
} } The Cl in tap water could lead to corrosion of metal in contact with the
} } water. A good additive IMO is Ethylene Glycol as a 10% mix. I use
} } technical grade EG and add 1/2 gallon to the 4.5 gallons of distilled
} } water for 5 gallons total in the Haskris R050 chiller reservoir.
} }
} } Sometimes this holds up for a year.
} }
} } gary g.
} }
} }
} }
} } At 04:52 AM 1/10/2008, you wrote:
} }
} }
} }
} }
} }
} } } -----------------------------------------------------------------------
} } } ----- The Microscopy ListServer -- CoSponsor: The Microscopy Society
} } } of America To Subscribe/Unsubscribe --
} } } http://www.microscopy.com/MicroscopyListserver
} } } On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} } } -----------------------------------------------------------------------
} } } -----
} } }
} } } Hi!
} } } During some works in a room next to our TEM, one worker opened a
} } } canalisation of the watercooling system, emptying the water tank of the
} } }
} } } watercooling device.
} } } I filled it again with normal tap water but I think I have to add some
} } } product to avoid mold growth.
} } } Could you recommend one such product and where I can order it,
} } } especially those of you from Germany and Austria (we are located in
} } } Vienna, Austria)?
} } } Our microscope is a Tecnai G20 and the watercooling unit is a Zephy ZEM
} } }
} } 1000S.
} }
} } } Thank you in advance,
} } } Stephane
} } }
} } ==============================Original
} } Headers==============================
} } 11, 20 -- From gary-at-gaugler.com Thu Jan 10 16:56:56 2008 11, 20 --
} } Received: from qsmtp4.mc.surewest.net (qsmtp.mc.surewest.net
} } [66.60.130.145])
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} } id m0AMutZj015411
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} } 16:56:56 -0600
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} } Date: Thu, 10 Jan 2008 14:56:53 -0800 11, 20 -- To: nizets2-at-yahoo.com
} } 11, 20 -- From: Gary Gaugler {gary-at-gaugler.com} 11, 20 -- Subject: Re:
} } [Microscopy] Product for watercooling 11, 20 -- Cc: MSA listserver
} } {microscopy-at-microscopy.com} 11, 20 -- In-Reply-To:
} } {200801101252.m0ACqLYm004944-at-ns.microscopy.com}
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} }
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} }
} } ==============================Original Headers==============================
} } 25, 24 -- From a.d.mckinnon-at-abdn.ac.uk Fri Jan 11 09:47:45 2008
} } 25, 24 -- Received: from mailhub3.abdn.ac.uk (mailhub3.abdn.ac.uk
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} } 25, 24 -- Date: Fri, 11 Jan 2008 15:45:11 -0000
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} } 25, 24 -- From: "Mckinnon, Alastair D." {a.d.mckinnon-at-abdn.ac.uk}
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} ==============================Original Headers==============================
} 8, 21 -- From donovan-at-uoregon.edu Fri Jan 11 10:37:25 2008
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From: modla-at-dbi.udel.edu
Date: Fri, 11 Jan 2008 17:30:39 -0600
Subject: [Microscopy] viaWWW: TEM Recommendations

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Email: modla-at-dbi.udel.edu
Name: Shannon Modla

Organization: University of Delaware

Title-Subject: [Filtered] TEM Recommendations

Question:
I work in a multi-user bio-imaging facility, and we recently were funded to purchase a new TEM. We are interested in a TEM that is EM tomography capable with a high resolution CCD camera and is user-friendly. We plan to upgrade to include a cryo-stage in the near future, so an instrument that is cryo-ready would be beneficial.



I was wondering if anyone could provide me with recommendations for TEMs and their experience with tomography. Also, is there a good test sample that can be used to test EM tomography both with cryo and conventional preparations for the demos?



Sincerely,

Shannon


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From: mckee-at-helix.mgh.harvard.edu
Date: Fri, 11 Jan 2008 17:30:59 -0600
Subject: [Microscopy] viaWWW: service for older Reichert Ultrqacut E ultramicrotomes

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Email: mckee-at-helix.mgh.harvard.edu
Name: Mary McKee

Organization: MGH

Title-Subject: [Filtered] service for older Reichert Ultrqacut E ultramicrotomes

Question: We have 2 older (not ancient) working Ultracut E ultramicrotomes that we would like to have routine service on (cleaning, lubricating, etc). Leica will not service them any longer. Does anyone know of an independent person for the northeast region (Boston)? Thanks in advance.

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From: alissa.susanne-at-gmail.com
Date: Fri, 11 Jan 2008 17:31:25 -0600
Subject: [Microscopy] viaWWW: specimen preparation

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Email: alissa.susanne-at-gmail.com
Name: Alissa H

Organization: University of Maryland

Title-Subject: [Filtered] specimen preparation

Question: We have a new Zeiss AxioImager here, and I've been given the task of not only learning how to use it, but also one of my main projects involves use of the microscope to evaluate fluorescence of some bacteria.
I've transformed a plasmid with YFP on it into some streptococcus. I can find the buggers, take a reasonable Z stack, and even deconvolve the image.

What I'd like to learn is better ways to prepare my samples, right now I've just been making wet mounts with saline. I'd also like to learn how to better use Zeiss' computer program that we got with the microscope. I don't find the program intuitive, like I do for most computer programs, and am getting frustrated.
If anyone can give me good suggestions on where I can read about these things, I'd really appreciate it. I feel like a total newbie, and I'm not quite sure where to go to get good information.

Many thanks,
Alissa

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From: tivol-at-caltech.edu
Date: Fri, 11 Jan 2008 18:56:10 -0600
Subject: [Microscopy] Re: viaWWW: TEM Recommendations

Contents Retrieved from Microscopy Listserver Archives
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On Jan 11, 2008, at 3:30 PM, modla-at-dbi.udel.edu wrote:

} I work in a multi-user bio-imaging facility, and we recently were
} funded to purchase a new TEM. We are interested in a TEM that is
} EM tomography capable with a high resolution CCD camera and is user-
} friendly. We plan to upgrade to include a cryo-stage in the near
} future, so an instrument that is cryo-ready would be beneficial.
}
}
}
} I was wondering if anyone could provide me with recommendations for
} TEMs and their experience with tomography. Also, is there a good
} test sample that can be used to test EM tomography both with cryo
} and conventional preparations for the demos?
}
Dear Shannon,
To a great extent, the type of instrument necessary depends on the
specimens for which you wish to do tomography. If, for example, you
want to look at bacterial cells, then you will need a higher voltage
than if you only wish to look at viruses or protein complexes. Our
lab has had a very good experience with FEI instruments. The Tecnai
T12, which, while not our primary tomographic instrument, has both
tomographic and cryo capabilities, is very reliable and user
friendly. It is an off-the-shelf, but very high-end TEM. It is
limited, however, to specimens thinner than a typical bacterium. Our
main instrument is a Tecnai TF30H Polara with all the bells and
whistles, most of which are necessary for electron cryo-tomography,
especially of whole bacterial cells. It has a field-emission source,
necessary for good beam coherence for phase contrast; it operates at
300 kV, which provides the penetrating power to observe ~0.5 um
specimens tilted to 70 degrees (an effective thickness of 1.5 um);
its cartridge system for holding specimens provides accurate and
reproducible tilting for good tracking during tilt-series data
collection; it has an energy filter, which provides increased
contrast and resolution by looking only at elastically scattered
electrons; and, finally, it is equipped with a 4k x 4k GATAN
Ultracam. It too is pretty reliable, but, being more complicated
than the T12, there are more things that can go wrong. The only
drawback to the Polara is its price, but I would hope that any
administrator who wants to get into the electron cryo-tomography
field would be willing to spend what is necessary. I would suggest
using a 250 nm conventional plastic section for a room temperature
test object and whatever is your favorite specimen--limited to a
thickness that suits the instrument--for a cryo test object.
Yours,
Bill Tivol, PhD
EM Scientist
Electron Cryo-Microscopy Facility
Broad Center, Mail Code 114-96
California Institute of Technology
Pasadena CA 91125
(626) 395-8833
tivol-at-caltech.edu


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From: r.kirk-at-kingston.ac.uk
Date: Sun, 13 Jan 2008 09:32:32 -0600
Subject: [Microscopy] AskAMicroscopist: SEM of protists

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Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (r.kirk-at-kingston.ac.uk) from http://microscopy.com/Ask-A-Microscopist/Ask-A-Microscopist.html on Sunday, January 13, 2008 at 07:07:47
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Email: r.kirk-at-kingston.ac.uk
Name: Dr Ruth Kirk

Organization: Kingston University

Education: Undergraduate College

Location: Surrey, UK

Question: I am currently supervising a student project which will investigate the use of different types of preparation techniques for SEM of protists. Do you have any advice on aggregating the protists during processing? That is, can you stick them to a cover slip or similar?

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From: panxijiang-at-gmail.com
Date: Sun, 13 Jan 2008 11:46:10 -0600
Subject: [Microscopy] viaWWW: bake out" procedure on the FEI CM series TEM

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Email: panxijiang-at-gmail.com
Name: Xijiang Pan

Organization: Tsinghua University

Title-Subject: [Filtered] how to perform "bake out" procedure on the FEI CM series TEM

Question: I am wondering if there is anybody in this list farmiliar with the "bake out" procedure for the FEI CM serious TEM. The local service engineers do not have any experiences in such work. So if you know,please contact me. Thanks in advance.

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From: kraftpiano-at-gmail.com
Date: Sun, 13 Jan 2008 12:49:48 -0600
Subject: [Microscopy] Product for watercooling

Contents Retrieved from Microscopy Listserver Archives
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Just out of curiosity, since a chiller is a relatively closed system,
what about putting a dilute chlorine solution in, like that used in
pools? Or perhaps a slight bleach additive? Would that damage the
equipment?

--Justin A. Kraft

On Jan 11, 2008 12:05 PM, {bbandli-at-mvainc.com} wrote:
}
}
}
} ----------------------------------------------------------------------------
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of America
} To Subscribe/Unsubscribe -- http://www.microscopy.com/MicroscopyListserver
} On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} ----------------------------------------------------------------------------
}
} I second John's "solution". It's what we have been using for our FESEM
} for several years without any problems. Opaque lines from the chiller
} to the scope are essential however. Even though this is what this scope
} has been on since day 1, we do have a small amount of rust/grit in the
} bottom of the tank but it hasn't been a problem. We also change the H2O
} every 6months (Per JEOL service).
} Cheers,
} Bryan Bandli
}
} donovan-at-uoregon.edu wrote:
} } ----------------------------------------------------------------------------
} } The Microscopy ListServer -- CoSponsor: The Microscopy Society of America
} } To Subscribe/Unsubscribe -- http://www.microscopy.com/MicroscopyListserver
} } On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} } ----------------------------------------------------------------------------
} }
} } All,
} } After much fighting of corrosion and algae issues I settled years ago
} } on what might be the easiest and most long term "solution". That is
} } pure distilled water. And here's the secret, you don't need to add
} } any chemical additives if you remove all clear plastic hoses from the
} } system and replace them with black or otherwise opaque materials. No
} } light, no growth.
} }
} } With this "solution" I have found I can run for years with a crystal
} } clear tank and with only an occasional speck of rust visible in the
} } bottom of the tank, which is probably left over from the prior years
} } of running god know what through the lines. This "solution" is
} } currently running in several SEMs and microprobes, using a variety of
} } chillers (mostly Haskris which I have found to be much more reliable
} } than Coolwell).
} }
} } Works for me anyway.
} } john
} }
} } At 07:58 AM 1/11/2008, a.d.mckinnon-at-abdn.ac.uk wrote:
} }
} }
} }
} }
} } } ----------------------------------------------------------------------------
} } } The Microscopy ListServer -- CoSponsor: The Microscopy Society of America
} } } To Subscribe/Unsubscribe -- http://www.microscopy.com/MicroscopyListserver
} } } On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} } } ----------------------------------------------------------------------------
} } }
} } } Hi,
} } }
} } } We incorporate Sigma water bath treatment in the reservoir - 3.5ml per
} } } tank full (25L).
} } }
} } } Seems to work well - lasting about 12 months and got this recommendation
} } }
} } } from Sigma Technical Services re using it in chiller circulators for
} }
} } } EMs.
} } }
} } } TechServ_Number: S5525
} } } TechServ_Name: SigmaClean; water bath treatment
} } } TechServ_Brand: SIGMA
} } }
} } } TechServ_re: is this product recommended for use in chiller circulators
} } } for
} } } the supply of cooling water for a transmission EM (Philips CM10).
} } }
} } } Best regards,
} } }
} } } Alastair
} } }
} } } Alastair McKinnon
} } } Histology & EM Facility Manager, IMS R2.62
} } } University of Aberdeen, Institute of Medical Science
} } } Foresterhill, Aberdeen, AB25 2ZD
} } } tel: +44(0)1224 552923 (office); +44(0)1224 555911 (lab)
} } } fax: +44(0)1224 559533; email: a.d.mckinnon-at-abdn.ac.uk
} } } www.abdn.ac.uk/ims/h-em
} } } -----Original Message-----
} } } X-from: gary-at-gaugler.com [mailto:gary-at-gaugler.com]
} } } Sent: 10 January 2008 23:00
} } } To: Mckinnon, Alastair D.
} } } Subject: [Microscopy] Re: Product for watercooling
} } }
} } }
} } }
} } }
} } } ------------------------------------------------------------------------
} } } ----
} } } The Microscopy ListServer -- CoSponsor: The Microscopy Society of
} } } America To Subscribe/Unsubscribe --
} } } http://www.microscopy.com/MicroscopyListserver
} } } On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} } } ------------------------------------------------------------------------
} } } ----
} } }
} } } I would suggest draining the water and replacing with distilled water.
} } } The Cl in tap water could lead to corrosion of metal in contact with the
} } } water. A good additive IMO is Ethylene Glycol as a 10% mix. I use
} } } technical grade EG and add 1/2 gallon to the 4.5 gallons of distilled
} } } water for 5 gallons total in the Haskris R050 chiller reservoir.
} } }
} } } Sometimes this holds up for a year.
} } }
} } } gary g.
} } }
} } }
} } }
} } } At 04:52 AM 1/10/2008, you wrote:
} } }
} } }
} } }
} } }
} } }
} } } } -----------------------------------------------------------------------
} } } } ----- The Microscopy ListServer -- CoSponsor: The Microscopy Society
} } } } of America To Subscribe/Unsubscribe --
} } } } http://www.microscopy.com/MicroscopyListserver
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} } } } -----------------------------------------------------------------------
} } } } -----
} } } }
} } } } Hi!
} } } } During some works in a room next to our TEM, one worker opened a
} } } } canalisation of the watercooling system, emptying the water tank of the
} } } }
} } } } watercooling device.
} } } } I filled it again with normal tap water but I think I have to add some
} } } } product to avoid mold growth.
} } } } Could you recommend one such product and where I can order it,
} } } } especially those of you from Germany and Austria (we are located in
} } } } Vienna, Austria)?
} } } } Our microscope is a Tecnai G20 and the watercooling unit is a Zephy ZEM
} } } }
} } } 1000S.
} } }
} } } } Thank you in advance,
} } } } Stephane
} } } }
} } } ==============================Original
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} } } 11, 20 -- From gary-at-gaugler.com Thu Jan 10 16:56:56 2008 11, 20 --
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} } } 11, 20 -- From: Gary Gaugler {gary-at-gaugler.com} 11, 20 -- Subject: Re:
} } } [Microscopy] Product for watercooling 11, 20 -- Cc: MSA listserver
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} } 8, 21 -- Subject: Re: [Microscopy] Product for watercooling
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From: colijn.1-at-osu.edu
Date: Sun, 13 Jan 2008 14:04:17 -0600
Subject: [Microscopy] Re: Product for watercooling

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Justin,

While chlorine bleach will kill most stuff, at least one chiller
manufacturer (Haskris) says that more than ~7ppm free Cl will damage
the buna-N O-ring seals. I worked it out a few years ago and figured
that it was ~50ml of household bleach in our chiller tank.

We have occasionally done a shock treatment with a high concentration
of bleach to kill stuff in the tank, then flushed it out. We've not
had any trouble with the seals so far. Minimizing the amount of
light that gets to the water makes a real difference in the amount of
gunk that develops.

Cheers,
Henk


At 01:51 PM 1/13/2008, kraftpiano-at-gmail.com wrote:



} ----------------------------------------------------------------------------
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of America

Hendrik O. Colijn colijn.1-at-osu.edu
OSU Campus Electron Optics Facility (614) 292-0674
040 Fontana Labs, 116 W. 19th Ave www.ceof.ohio-state.edu


==============================Original Headers==============================
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11, 26 -- Subject: Re: [Microscopy] Product for watercooling
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From: PRICE-at-gw.med.sc.edu
Date: Mon, 14 Jan 2008 07:05:04 -0600
Subject: [Microscopy] viaWWW: Basic Confocal Microscopy and Digital Imaging Workshop

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

This Question/Comment was submitted to the Microscopy Listserver
using the WWW based Form at http://microscopy.com/MLFormMail.html
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Email: PRICE-at-gw.med.sc.edu
Name: Bob Price

Organization: USC- School of Medicine

Title-Subject: [Filtered] Basic Confocal Microscopy and Digital Imaging Workshop

Question: Dear List Members,

Appended below is information about our fourth Basic Confocal
Microscopy and Digital Imaging Workshop that will be held at the
University of South Carolina School of Medicine from June 16-20, 2008.


Workshop on Basic Confocal Microscopy and Digital Imaging: Brief
Synopsis

The South Carolina EPSCoR/IDeA Program and the USC School of Medicine
Instrumentation Resource Facility are pleased to announce the 4th
annual
workshop on Basic Confocal Microscopy and Digital Imaging. The
hands-on
workshop will target beginning and intermediate users of confocal
microscopes and will provide lectures from experts in the field of
confocal microscopy and the use of Adobe Photoshop and 3-D software
for
processing of confocal images. Lecture material will provide
information
on the basics of fluorescence and fluorescent probes, biological
specimen preparation (fixation, staining, optical properties and
mounting materials), strategies and protocols for selection of
antibody
labeling, the basic components of a confocal microscope (lasers,
dichroic mirrors, microscope objectives, photomultiplier tubes, etc.)
and an overview of some applications of confocal microscopy.

During the laboratory portion of the workshop specimens will be
processed for double and triple labeling and proper selection of user
adjustable parameters to optimize image collection will be addressed
and
demonstrated. Participants are welcome to process their own samples
or
to use samples that will be provided. Several point scanning and
spinning disk confocal systems from various manufacturers will be
available for use so participants will have ample time for hands on
use
of the instruments during the workshop.

Faculty scheduled to participate include:

Dr. Bob Price, Research Professor, Cell and Developmental Biology and
Anatomy, and Director, Instrumentation Resource Facility, University
of
South Carolina School of Medicine
(http://dba.med.sc.edu/price/irf/irf.htm)
Dr. Jay Jerome, Associate Professor, Pathology and Cancer Biology,
Vanderbilt University
(https://medschool.mc.vanderbilt.edu/facultydata/php_files/show_faculty.php?id3=1032)
Dr. Ralph Albrecht, Professor, Department of Animal Sciences,
University of Wisconsin-Madison
(http://www.ansci.wisc.edu/facstaff/Faculty/pages/albrecht/index.htm)
Dr. John Mackenzie, Professor, Microbiology, North Carolina State
University (http://www.ncsu.edu/cem/index.html)
Dr. Tom Trusk, Associate Professor, Department of Cell Biology and
Anatomy, Medical University of South Carolina
(http://cba.musc.edu/faculty/TruskT.htm)


Past workshops have been very successful with over 50 attendees at
each. For further information contact Bob Price (Price-at-med.sc.edu) or
visit the workshop website: http://dba.med.sc.edu/price/irf/irf.htm

Robert L. Price, PhD
Research Professor and
Director, Instrumentation Resource Facility
School of Medicine, USC
Bldg 1 Room B60
6439 Garner's Ferry Road
Columbia, SC 29208

Fax: 803-733-1533
Telephone: 803-733-3392



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19, 11 -- From zaluzec-at-microscopy.com Mon Jan 14 07:05:03 2008
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From: nizets2-at-yahoo.com
Date: Mon, 14 Jan 2008 08:11:50 -0600
Subject: [Microscopy] viaWWW: specimen preparation

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi!

Perhaps it would comfort you to know that I have exactly the same feeling with our Zeiss axiovert.
The microscope itself is well designed but the software is user-unfriendly. The main operations, those obligatory steps that you use all the time are dispersed in different commands and subcommands. I constantly feel that I am using only 0,1% of the possibilities of the system, without hope of increasing this percentage.
The best answer I can give you is to arrange a course with Zeiss.

Best regards,
Stephane

PS: Z-stack on bacteria with a light microscope?? Are you sure you are not talking about confocal?

----- Original Message ----
X-from: "alissa.susanne-at-gmail.com" {alissa.susanne-at-gmail.com}
To: nizets2-at-yahoo.com
Sent: Saturday, January 12, 2008 12:38:35 AM

This Question/Comment was submitted to the Microscopy Listserver
using the WWW based Form at http://microscopy.com/MicroscopyListserver/MLFormMail.html
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Email: alissa.susanne-at-gmail.com
Name: Alissa H

Organization: University of Maryland

Title-Subject: [Filtered] specimen preparation

Question: We have a new Zeiss AxioImager here, and I've been given the task of not only learning how to use it, but also one of my main projects involves use of the microscope to evaluate fluorescence of some bacteria.
I've transformed a plasmid with YFP on it into some streptococcus. I can find the buggers, take a reasonable Z stack, and even deconvolve the image.

What I'd like to learn is better ways to prepare my samples, right now I've just been making wet mounts with saline. I'd also like to learn how to better use Zeiss' computer program that we got with the microscope. I don't find the program intuitive, like I do for most computer programs, and am getting frustrated.
If anyone can give me good suggestions on where I can read about these things, I'd really appreciate it. I feel like a total newbie, and I'm not quite sure where to go to get good information.

Many thanks,
Alissa

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____________________________________________________________________________________
Never miss a thing. Make Yahoo your home page.
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From: bigelow-at-umich.edu
Date: Mon, 14 Jan 2008 15:19:40 -0600
Subject: [Microscopy] RE: Algaecides

Contents Retrieved from Microscopy Listserver Archives
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I agree about the opaque lines but found it much easier to use normal
transparent hoses and wrap them in aluminium foil with a bit of tape.
It's worked for years on our SEM.

Malcolm

Malcolm Haswell
e.m. unit
Chemispec
School of Health, Natural and Social Sciences
Fleming Building
University of Sunderland
Tyne & Wear
SR1 3SD
UK
e-mail: malcolm.haswell-at-sunderland.ac.uk



----- Original Message -----
X-from: bbandli-at-mvainc.com

Preventing the growth of algae in cooling water systems is discussed
in detail in my book "Vacuum Methods in Electron Microscopy" Two
chemicals commonly used to prevent algal growth in such systems are
Chloramine T and dichlorophene. Both of these chemicals can be
obtained from various specialty chemical companies. You can also
probably obtain algaecides from companies (and merchants) that sell
water beds, and swimming pool equipment. I do not recommend the use
of ethylene glycol for several reasons that are discussed in my book.
Also, remember that algae require light in order to grow, and so you
can substantially inhibit their growth by fully excluding light from
the system (i.e. cover the reservoir with a a light-tight cover, and
use fully opaque tubing). Changing from ordinary tap water to
distilled water will probably not give you much of an advantage,
except for possibly minimizing the formation of a bit of scale in the
heated parts of the diffusion pump. However, the amount of scale
formation should be quite limited since it is a closed system
containing a limited amount of water.
--
Wilbur C. Bigelow, Professor Emeritus
Materials Sci. & Engr., Univ. of Michigan
Ann Arbor, Michigan 48109-2136
e-mail: bigelow-at-umich.edu;
Fx:734-763-4788; Ph:734-975-0858
Address mail to: 2911 Whittier Court
Ann Arbor, MI 48104-6731

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From: slc6-at-lehigh.edu
Date: Mon, 14 Jan 2008 18:07:05 -0600
Subject: [Microscopy] viaWWW: Lehigh Microscopy School Courses

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Email: slc6-at-lehigh.edu
Name: Sharon Coe

Organization: Lehigh Microscopy School

Title-Subject: [Filtered] Lehigh Microscopy School Courses

Question: There is still time to register for the 2008 Lehigh Microscopy School which will be held June 1-13, 2008. This will be the 38th year of course offerings which include:

SEM and X-Ray Microanalaysis (June 2-6)

Introduction to SEM and EDS for the New Operator (June 1)

Scanning Probe Microscopy: From Fundamentals to Advanced Applications (June 9-12)

Problem Solving with SEM, X-ray Microanalysis, and Electron Backscatter Patterns (June 9-13)

Quantitative X-ray Microanalysis: Problem Solving Using EDS and WDS Techniques (June 9-13)

Analytical Electron Microscopy at the Nanometer Scale
(June 9-12)

Focused Ion Beam (FIB) Instrumentation and Applications (June 9-12)

Complete course descriptions and registration form are available at www.Lehigh.edu/microscopy. Contact Sharon Coe (Sharon.coe-at-Lehigh.edu) for more information.

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From: a.c.richardson-at-durham.ac.uk
Date: Tue, 15 Jan 2008 07:18:39 -0600
Subject: [Microscopy] TEM : AFS problem

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Dear Microscopists,

Has anyone encountered problems with fumes escaping from specimen chamber of a
Leica Freeze substitution unit ( AFS not AFS2.) during fluid changes.

A new user has noticed, especially when doing changes with Lowicryl HM20, that
the fumes are escaping and therefore it is putting the user at risk and others
who may be in the area at the time.The built in venting system of the AFS is
ducted into a fume hood and appears to be working, at least we can feel air
movement from it. Is it possible the fan is not working efficiently ?

In the short term, though not ideal, we are dealing with this by providing users
with suitable respirator masks. A more long term/safer solution we are looking
into is to have some sort of extract system that will draw fumes away from the user.

If you have encountered this problem before how did you overcome it?

Christine Richardson.

School of Biological & Biomedical Science
Centre for Molecular Imaging
University of Durham
UK.

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From: vilde1-at-oslo.westerngeco.slb.com
Date: Tue, 15 Jan 2008 10:23:34 -0600
Subject: [Microscopy] Job opening : Failure Analysis Engineer based in Oslo, Norway

Contents Retrieved from Microscopy Listserver Archives
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Hello,

here is a description of the position. Please contact me for further inquiries.

Thanks and best regards,

Loic Vilde

Failure Analysis Engineer

Description :

You will apply your scientific and analytical
skills to assist in improving product reliability
through methodical root cause analysis of failed products.

Your responsibilities will include to design,
plan and lead all the investigations necessary to
identify the root cause of failed products (field
returns or test samples). You will approve,
archive and distribute the associated documentation.

You will also work on developing and implementing
new investigative procedures specifically aimed
at our designs and on organizing failure analysis
conclusions in a knowledge database. Our products
use diverse materials, from thermoplastics to
Titanium parts, with a special emphasis on
microelectronics components and printed circuit boards.

You will interface with the Product Development
Team members and Manufacturing engineers, as well
as with other Environmental Qualification
engineers and technical experts from other
Schlumberger Technology Centres, and external failure analysis labs.

Equipment used onsite to perform these
investigations includes: cold mounting station,
dye, precision cut-off machine, semi-automatic
grinder/polisher, carbon coater, optical
microscopes, variable pressure scanning electron
microscope (VP-SEM) with energy-dispersive X-Ray
microanalysis (EDS) and X-ray inspection system (Non-Destructive Testing).

Technical, product development, quality
management and business related training will be provided.

Notes : International Candidates Will Be
Considered. Employer will assist with relocation costs

Requirements :

Education and Qualifications:
* PhD in Material Science or MSc with working
experience in Failure Analysis domain
* Minimum 3 years working experience in similar field
* English (working language)
Expertise in one or several of the below domains will be highly appreciated :
* Scientific/technical experimentation and methods
* Analytical investigation procedures,
especially sample preparation for SEM/EDS
analysis of microelectronics components and electronic assemblies
Others :
* Ability to organize and document investigations
* Strong SEM/EDS and sample preparation skills
* Team player with open and direct communication style
* Solid computer skills/literacy, especially in data analysis
* Effective oral and written communication skills
Employer :

{http://www.westerngeco.com/} Schlumberger
WesternGeco {http://www.westerngeco.com/}

WesternGeco, the world's largest geophysical
services company, provides comprehensive
worldwide reservoir imaging, monitoring, and
development services, with the most extensive
geophysical survey crews and data processing
centers in the industry, as well as the world's
largest multiclient data library. Services range
from 3D and time-lapse (4D) seismic surveys to
multicomponent surveys for delineating prospects
and reservoir management as well as electromagnetic surveys.



Loïc VILDE
Environmental Qualification / Test and Integration Manager
-------------------------------------------------------------
WesternGeco - Oslo Technology Center
Schlumberger House
Solbråveien 23
N-1372 Asker – Norway

Phone: +47 6678 8314
Fax: +47 6678 8500
E-Mail : vilde1-at-oslo.westerngeco.slb.com



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From: mckee-at-helix.mgh.harvard.edu
Date: Tue, 15 Jan 2008 13:32:20 -0600
Subject: [Microscopy] viaWWW: Thanks - service for microtomes

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Email: mckee-at-helix.mgh.harvard.edu
Name: Mary McKee

Organization: MGH

Title-Subject: [Filtered] service for microtomes

Question: Thanks to everyone who responded to my question. You are great!

Mary

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From: sandeep-at-frontedgetechnology.com
Date: Tue, 15 Jan 2008 21:31:38 -0600
Subject: [Microscopy] viaWWW: Scanning Electron Microscope Repair & Maintenance

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Email: sandeep-at-frontedgetechnology.com
Name: Sandeep

Organization: Front Edge Technology

Title-Subject: [Filtered] Scanning Electron Microscope Repair & Maintenance

Question: Hello All,

We require repair and maintenance services for the SEM & X-ray detector. Please recommend the service providers. We are located in Southern California.

Thank you & Regards.




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From: MILLERS-at-AGR.GC.CA
Date: Wed, 16 Jan 2008 15:07:25 -0600
Subject: [Microscopy] LM/Confocal- need help identifying plant organelles

Contents Retrieved from Microscopy Listserver Archives
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Hi all;

One of my users has been doing some subcellular fractionation of plant cells, and would like to look at the fractions to see if we can identify specific organelles. Are there any specific probes that will help us? I would appreciate any advice! We do have a confocal microscope, which should give us better resolution than a std fluorescence microscope.



Thanks in advance

shea

Dr. S. Shea Miller
Agriculture and Agri-Food Canada/Agriculture et Agroalimentaire Canada
Telephone/Téléphone: 613-759-1760
Facsimile/Télécopieur: 613-759-1701
Rm 2068 K.W. Neatby Bldg
960 Carling Ave.
Central Experimental Farm
Ottawa, ON
K1A 0C6
millers-at-agr.gc.ca
 




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From: jason_jla-at-hotmail.com
Date: Wed, 16 Jan 2008 19:04:36 -0600
Subject: [Microscopy] AskAMicroscopist: where to purchase a good microscope that can

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Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (jason_jla-at-hotmail.com) from http://microscopy.com/Ask-A-Microscopist/Ask-A-Microscopist.html on Wednesday, January 16, 2008 at 11:53:09
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Email: jason_jla-at-hotmail.com
Name: Jason Alexander

Organization: Immanuel-St. James

Education: K-8 Grade Grammar School

Location: Grand Rapids, MI

Question: Where can I purchase a good microscope that can be used for CELLS and MICROSTRUCTURES OF METALLIC SPECIMENS? I am writing a grant for a microscope and the organization recommended I ask you this question. Thank you for your time?


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From: john.d.williams-at-colostate.edu
Date: Wed, 16 Jan 2008 19:05:27 -0600
Subject: [Microscopy] AskAMicroscopist: Questions on an ISI-DS130S

Contents Retrieved from Microscopy Listserver Archives
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This Question was submitted to Ask-A-Microscopist by (john.d.williams-at-colostate.edu)
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Email: john.d.williams-at-colostate.edu
Name: Prof. John D. Williams

Organization: Colorado State University

Education: Graduate College

Location: Fort Collins, Colorado, USA

Title: Questions on an ISI-DS130S

Question: I'm being offered a scanning microscope as a donation. It is an ISI-DS130S and was in good working order 2 years ago before being crated up. Does anyone have any detailed information on this scope? I just need a good workhorse for inspecting heavily ion etched surfaces. The last significant contact I've had with an SEM was with Bob Lee at CSU in the late 1980s. So everyone should consider me a newbie. Thanks.

---------------------------------------------------------------------------

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From: john.d.williams-at-colostate.edu
Date: Wed, 16 Jan 2008 22:11:24 -0600
Subject: [Microscopy] AskAMicroscopist: ISI-DS130S operating/maintenance manual

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This Question was submitted to Ask-A-Microscopist by (john.d.williams-at-colostate.edu)
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Email: john.d.williams-at-colostate.edu
Name: Prof. John D. Williams

Organization: Colorado State University

Education: Graduate College

Location: Fort Collins, Colorado, USA

Title: ISI-DS130S

Question: Does anyone have an ISI-DS130S operating/maintenance manual they would be willing sell/give me? Thanks, John Williams

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From: stefan.diller-at-t-online.de
Date: Thu, 17 Jan 2008 05:35:29 -0600
Subject: [Microscopy] Thanks to the list... Follow-up: calendar text in english language

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Follow-up:
I am grateful to Maryah Converse, daughter of Ken Converse of
www.qualityimages.biz for translating the descriptions of the images of my
SEM calendar "Microstructures 2008". All texts on page 14 are now in English
language.

If anybody is able to put the complete calendar PDF
www.elektronenmikroskopie.info/calendar_2008.pdf (39 MB)
on a server with unrestricted traffic, please do so and let the list know. I
will take the file off my server within 12 hours, because I spend all my
free transfer volume for this month on my server ;-(
If you would only like to get the updated page 14 with the English text,
this is the place:
www.elektronenmikroskopie.info/calendar_2008_p14.pdf (350 KB)

Best regards,
Stefan




}
} Dear All,
} thanks for the good discussion and the helpful tips to all on the list.
}
}
} With the best wishes for a
} happy new year 2008,
} success at work and in business,
}
} Stefan Diller
}
}
}
} Please feel free to download and print out my new SEM Calendar 2008
} with images from scanning electron microscopy:
} www.elektronenmikroskopie.info/calendar_2008.pdf (39 MB). Images are
} Copyright Stefan Diller 2008, please ask for permission prior to any
} commercial use.
}

----------------------------------------------------------------------------
-----------------------------------------
Stefan Diller - Scientific Photography
Arndtstrasse 22
D - 97072 Wuerzburg Germany
++49 - 931 - 7848700 Phone
++49 - 931 - 7848701 Fax
++49 - 175 - 717 70 51 Cell-Phone

Websites:
www.stefan-diller.com
www.elektronenmikroskopie.info
www.assisi.de
www.zwillingsprojekt.de
Anfahrt: http://mail.map24.com/stefan.diller
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From: beth-at-plantbio.uga.edu
Date: Thu, 17 Jan 2008 10:21:22 -0600
Subject: [Microscopy] sectioning watermelon seeds

Contents Retrieved from Microscopy Listserver Archives
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Hi all,
Happy New Year!
Does anyone have experience thick-sectioning watermelon seeds? We're
working with mature seeds - black seed coat - unfixed, not embedded.
The seeds are left in a moist chamber overnight to imbibe water.
Vibratome sectioning didn't work well. Any suggestions? Would fixing
and embedding make them easier to section?

I think they're really only good for spitting...but the researcher
doesn't want to hear that;-)
Any help would be greatly appreciated.
Many thanks,
Beth

Beth Richardson
Plant Biology Department
University of Georgia
Athens, GA 30602
706-542-1790


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From: pekysar-at-ucdavis.edu
Date: Thu, 17 Jan 2008 10:28:28 -0600
Subject: [Microscopy] SEM of Wires Encased in Polyurethane

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hello All,
I have a researcher who wants to look at polyurethane coated wires with the
SEM. His goal is to see any cracks, breaks or defects in the metal wire
encased by the polyurethane. These are very tiny wires, he cannot remove the
covering and he needs to look at the wire in sections for defects. We have a
super SEM with a backscatter detector but no carbon coater. Any one have
experience with this type of sample? How can I prep the samples for the
SEM?? Any suggestions would be greatly appreciated!! Thanks!
Pat Kysar
University of California, Davis
Medical School, Pathology
EM Lab



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From: stefan.diller-at-t-online.de
Date: Thu, 17 Jan 2008 11:17:27 -0600
Subject: [Microscopy] Thanks to the list... Follow-up: calendar text in english language -new address

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Dear All,
thanks to Kay at www.quantifoil.com at Jena, Germany
the calendar PDF finally moved on to this download address:
www.quantifoil.com/calendar_2008.pdf (38 MB)
It will be available hopefully the rest of 2008.

If you would only like to get the updated page 14 with the English text, it
will stay available here:
www.elektronenmikroskopie.info/calendar_2008_p14.pdf (350 KB)

Best regards,
Stefan





----------------------------------------------------------------------------
-----------------------------------------
Stefan Diller - Scientific Photography
Arndtstrasse 22
D - 97072 Wuerzburg Germany
++49 - 931 - 7848700 Phone
++49 - 931 - 7848701 Fax
++49 - 175 - 717 70 51 Cell-Phone

Websites:
www.stefan-diller.com
www.elektronenmikroskopie.info
www.assisi.de
www.zwillingsprojekt.de
Anfahrt: http://mail.map24.com/stefan.diller
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From: gnord-at-mindspring.com
Date: Thu, 17 Jan 2008 11:19:54 -0600
Subject: [Microscopy] Re: SEM of Wires Encased in Polyurethane

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Visit the Geology Department at Davis. They will have a carbon coater.

On Jan 17, 2008, at 11:28 AM, pekysar-at-ucdavis.edu wrote:

}
}
}
} ----------------------------------------------------------------------
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} The Microscopy ListServer -- CoSponsor: The Microscopy Society of
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} MicroscopyListserver
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}
} Hello All,
} I have a researcher who wants to look at polyurethane coated wires
} with the
} SEM. His goal is to see any cracks, breaks or defects in the metal
} wire
} encased by the polyurethane. These are very tiny wires, he cannot
} remove the
} covering and he needs to look at the wire in sections for defects.
} We have a
} super SEM with a backscatter detector but no carbon coater. Any one
} have
} experience with this type of sample? How can I prep the samples for
} the
} SEM?? Any suggestions would be greatly appreciated!! Thanks!
} Pat Kysar
} University of California, Davis
} Medical School, Pathology
} EM Lab
}
} ---------------------------------

Gordon L. Nord, Ph. D
Senior Scientist
International Environmental Research Foundation
New York, NY

{http://www.ierfinc.org/}

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From: ALawrence-at-entomology.msstate.edu
Date: Thu, 17 Jan 2008 13:14:13 -0600
Subject: [Microscopy] M&M 2008 student bursary and volunteer request

Contents Retrieved from Microscopy Listserver Archives
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Greetings,
This is the first announcement for students who will attend the Microscopy and Microanalysis Meeting in Albuquerque, Aug.3-7 and would like to apply for a Student Bursary to help defray meeting costs. The complete description of the Bursary is listed below, including the registration process.

The contact person this year that will coordinate the initial student bursary sign-up is: Amanda Lawrence (alawrence-at-entomology.msstate.edu ). Clayton Lohen (clohen-at-vt.edu) will be helping with coordination of bursary activities once on site.

STUDENT BURSARIES
The Microscopy Society of America values student members and recognizes that they are the future of both the society and the field of microscopy in general. MSA is therefore pleased to offer student bursaries of $200 to registered students. The most important purpose of these bursaries is to encourage students to attend the annual MSA/MAS Microscopy and Microanalysis meeting, where these young scientists can meet and interact with the established microscopy community as well as assisting with the meeting.

Each bursary recipient will be expected to work for a minimum of 20 hours during the meeting and/or at the pre-meeting weekend events. A student may work up to an additional 20 hours, for a total of 40 hours. These extra hours will add to the bursary total at a rate of $10 per hour. The maximum bursary will therefore be $400. The duties will involve, but are not necessarily limited to, providing support in symposia (helping with audio-visual needs, maintaining an attendance count, and helping speakers set up for their presentation), staffing the MSA Megabooth, and monitoring use of the Internet Cafe. Applicants for the bursaries must be members of MSA or MAS, and enrolled as students at a recognized educational institution. All MSA or MAS student members are eligible for bursaries, including those who are recipients of MSA Presidential Scholars Awards and MAS Distinguished Scholar Awards. Eligible on the conference website, or at on-site registration. Bursaries are limited and early application is encouraged. Don't forget to check the website for special student housing discounts as well.

How it works:
The registration form for the meeting will have a check box indicating that the applicant is a registered student and is requesting a bursary. The check box will have a note beside it reminding the applicant that the bursary requires them to work at the meeting.

Students who have applied for bursaries will be contacted by the initial student bursary co-coordinator (Amanda) to schedule meeting tasks prior to arrival in Albuquerque. The student is then expected to fulfill their assigned tasks and will be issued forms which must be signed by all of the contact persons listed, indicating that all assigned tasks have been performed. Upon completion of assignments and submission of the signed forms, the bursary check will be issued by the appropriate LAC representative.

We would also like to solicit volunteers from 'non-students' as well to help with meeting activities.

Should you have questions , please contact:

Amanda Lawrence (alawrence-at-entomology.msstate.edu)
Electron Microscope Center
100 Twelve Lane
Mississippi State University
Mississippi State, MS 39762
(662)-325-3019 Work
(662)-325-0246 Fax





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From: gary.m.brown-at-exxonmobil.com
Date: Thu, 17 Jan 2008 14:42:52 -0600
Subject: [Microscopy] SEM of Wires Encased in Polyurethane

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Gordon,

I have several questions that may allow you to provide more specific
information useful to the listserver community: Is the polyurethane
cross-linked? Does he need to examine the wire in cross-section or might
examination of the surface of the wire suffice? If a cross-section is
required, which plane of the wire does he want to examine, i.e. the axial
cross-section or the longitudinal cross-section? How do you intend to
prepare the cross-sections: grinding and polishing; microtomy; FIB, etc?

If the polyurethane is not cross-linked, I suggest you consider dissolving
it in a good solvent, thus leaving the bare wires available for subsequent
sample preparation and microscopy.

Best regards,


Disclaimer: The comments and opinions given above are those of the author
alone and do not represent any position of ExxonMobil Chemical Company.


Gary M. Brown
Microscopy Specialist
ExxonMobil Chemical Company
Baytown Technology & Engineering - West
5200 Bayway Drive
Baytown, Texas 77520-2101
phone: 281 834 2387
fax: 281 834 2395
e-mail: Gary.M.Brown-at-ExxonMobil.com

"Our business in life is not to succeed, but to continue to fail in good
spirits." Robert Louis Stevenson






gnord-at-mindspri
ng.com
To
gary.m.brown-at-exxonmobil.com
01/17/08 11:21 cc
AM
Subject
[Microscopy] Re: SEM of Wires
Please respond Encased in Polyurethane
to
gnord-at-mindspri
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Visit the Geology Department at Davis. They will have a carbon coater.

On Jan 17, 2008, at 11:28 AM, pekysar-at-ucdavis.edu wrote:

}
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} Hello All,
} I have a researcher who wants to look at polyurethane coated wires
} with the
} SEM. His goal is to see any cracks, breaks or defects in the metal
} wire
} encased by the polyurethane. These are very tiny wires, he cannot
} remove the
} covering and he needs to look at the wire in sections for defects.
} We have a
} super SEM with a backscatter detector but no carbon coater. Any one
} have
} experience with this type of sample? How can I prep the samples for
} the
} SEM?? Any suggestions would be greatly appreciated!! Thanks!
} Pat Kysar
} University of California, Davis
} Medical School, Pathology
} EM Lab
}
} ---------------------------------

Gordon L. Nord, Ph. D
Senior Scientist
International Environmental Research Foundation
New York, NY

{http://www.ierfinc.org/}

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From: mgengle-at-uky.edu
Date: Thu, 17 Jan 2008 19:16:43 -0600
Subject: [Microscopy] viaWWW: Microwave processing for TEM

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Email: mgengle-at-uky.edu
Name: Mary Gail Engle

Organization: Imaging Facility, University of Kentucky

Title-Subject: [Filtered] Microwave processing for TEM

Question: Having just attended a microwave workshop and being impressed with the morphology of the tissue for "normal" EM, I was wondering if any of you have experience with, or an opinion regarding the quality of colloidal gold immunolabeling using the microwave.
Speed is not necessarily an issue for us, but if we could get better morphology as well as good gold labeling, we would consider purchasing the instrument.

Thank you,
Mary Gail Engle,
Manager, Imaging Facility
University of KY

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From: atn5613-at-rit.edu
Date: Thu, 17 Jan 2008 19:17:12 -0600
Subject: [Microscopy] viaWWW: Target glue for PSD

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Email: atn5613-at-rit.edu
Name: Algis N

Organization: Rochester Institute of Technology

Title-Subject: [Filtered] Target glue for PSD

Question: Hello All,
I am doing some research using a plasma sputtering device (VCR Group IBS TM200S)to sputter metals onto a substrate. What type of adhesive should I use to adhere the metal foil targets I will be using to the target holder? Should it be conductive and what contamination concerns should I be looking for? Thanks.
Algis

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From: npchong-at-northwestern.edu
Date: Fri, 18 Jan 2008 16:06:14 -0600
Subject: [Microscopy] SEM - resources for images of well-prepared E. coli?

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Pat,
I'm a little confused by "he needs to look at the wire in sections". If you
mean that the wire will be cross-sectioned, then advice has already been
given: mount, grind and polish. If, on the other hand, you mean that
short, perhaps specific, sections will be examined for surface defects on
the metal wire and "he cannot remove the covering", my question is: how
thick is the polyurethane insulation? If it's only a couple of microns
thick, try going to your maximum kV and see if the beam will penetrate the
insulation. BSE may give the best image, but SE might also work. If the
insulation is too thick for beam penetration, you're left with either
stripping or sectioning.

Ken Converse
owner

QUALITY IMAGES
Servicing Scanning Electron Microscopes
Since 1981
474 So. Bridgton Rd.
Bridgton, ME 04009
207-647-4348
Fax 207-647-2688
kenconverse-at-qualityimages.biz
qualityimages.biz



-----Original Message-----
X-from: pekysar-at-ucdavis.edu [mailto:pekysar-at-ucdavis.edu]
Sent: Thursday, January 17, 2008 11:31 AM
To: kenconverse-at-qualityimages.biz

Hello All,
I have a researcher who wants to look at polyurethane coated wires with the
SEM. His goal is to see any cracks, breaks or defects in the metal wire
encased by the polyurethane. These are very tiny wires, he cannot remove the
covering and he needs to look at the wire in sections for defects. We have a
super SEM with a backscatter detector but no carbon coater. Any one have
experience with this type of sample? How can I prep the samples for the
SEM?? Any suggestions would be greatly appreciated!! Thanks! Pat Kysar
University of California, Davis Medical School, Pathology EM Lab



==============================Original Headers==============================
3, 21 -- From pekysar-at-ucdavis.edu Thu Jan 17 10:28:28 2008
3, 21 -- Received: from warsaw.ucdavis.edu (warsaw.ucdavis.edu
[128.120.32.41])
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-0600
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-0800 (PST)
3, 21 -- Message-ID: {001701c85926$549f8970$22c5eda9-at-ucdsom.ucdavis.edu}
3, 21 -- From: "Pat Kysar" {pekysar-at-ucdavis.edu}
3, 21 -- To: "Microscopy Listserver" {microscopy-at-microscopy.com} 3, 21 --

Ken,

Unfortunately, many technologists are put in your position. That is, one
may be asked to analyze potentially complex, multi-component materials
without substantive guidance from the requestor, in areas outside one's
expertise, and with little help within our immediate technical community.

I encourage you to put some of the responsibility back onto the requestor.
He/she should be able to obtain information on the composition of the
polyurethane insulation from the manufacturer. If the requestor is not
willing to spend any time or effort to work the problem, just how important
can it be? The last point I would make regards the scope of your technical
capabilities. Specifically, do you have the sample preparation and
microscopy capabilities that will be needed in the analysis of this
material.

Best regards,

Disclaimer: The comments and opinions given above are those of the author
alone and do not represent any position of ExxonMobil Chemical Company.

Gary M. Brown
Microscopy Specialist
ExxonMobil Chemical Company
Baytown Technology & Engineering - West
5200 Bayway Drive
Baytown, Texas 77520-2101
phone: 281 834 2387
fax: 281 834 2395
e-mail: Gary.M.Brown-at-ExxonMobil.com

"Our business in life is not to succeed, but to continue to fail in good
spirits." Robert Louis Stevenson






kenconverse-at-qu
alityimages.bi
z To
gary.m.brown-at-exxonmobil.com
cc
01/18/08 02:55
PM Subject
[Microscopy] RE: SEM of Wires
Encased in Polyurethane
Please respond
to
kenconverse-at-qu
alityimages.bi
z











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Pat,
I'm a little confused by "he needs to look at the wire in sections". If
you
mean that the wire will be cross-sectioned, then advice has already been
given: mount, grind and polish. If, on the other hand, you mean that
short, perhaps specific, sections will be examined for surface defects on
the metal wire and "he cannot remove the covering", my question is: how
thick is the polyurethane insulation? If it's only a couple of microns
thick, try going to your maximum kV and see if the beam will penetrate the
insulation. BSE may give the best image, but SE might also work. If the
insulation is too thick for beam penetration, you're left with either
stripping or sectioning.

Ken Converse
owner

QUALITY IMAGES
Servicing Scanning Electron Microscopes
Since 1981
474 So. Bridgton Rd.
Bridgton, ME 04009
207-647-4348
Fax 207-647-2688
kenconverse-at-qualityimages.biz
qualityimages.biz



-----Original Message-----
X-from: pekysar-at-ucdavis.edu [mailto:pekysar-at-ucdavis.edu]
Sent: Thursday, January 17, 2008 11:31 AM
To: kenconverse-at-qualityimages.biz


Hello All,
I have a researcher who wants to look at polyurethane coated wires with the
SEM. His goal is to see any cracks, breaks or defects in the metal wire
encased by the polyurethane. These are very tiny wires, he cannot remove
the
covering and he needs to look at the wire in sections for defects. We have
a
super SEM with a backscatter detector but no carbon coater. Any one have
experience with this type of sample? How can I prep the samples for the
SEM?? Any suggestions would be greatly appreciated!! Thanks! Pat Kysar
University of California, Davis Medical School, Pathology EM Lab



==============================Original
Headers==============================
3, 21 -- From pekysar-at-ucdavis.edu Thu Jan 17 10:28:28 2008
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[128.120.32.41])
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m0HGSRFu017857
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3, 21 -- Message-ID: {001701c85926$549f8970$22c5eda9-at-ucdsom.ucdavis.edu}
3, 21 -- From: "Pat Kysar" {pekysar-at-ucdavis.edu}
3, 21 -- To: "Microscopy Listserver" {microscopy-at-microscopy.com} 3, 21 --

I have been using a Hitachi 4800 SEM to image E. coli bacteria, but am
not sure if what I've been seeing is representative of good fixation
or sample preparation.

So far I've used a number of different fixatives (both with and
without microwave assistance), the latest being 1% PFA, 1% GA, 50 mM
cacodylate, pH 7.4. I have not been using any osmium. My main concern
comes from the fact that the E. coli always look a bit bumpy and
textured, not smooth and featureless like the B. subtilis I have also
been imaging with more success. Also, I almost never see flagella.

My question is if anyone has recommendations for some resources in
which I could find high resolution images of high-quality E. coli
samples. When I try doing a Google Images search, or a quick look at
PubMed, the micrographs I find are of considerably less resolution
than I typically get with the Hitachi 4800 I've been using, so I'm
never sure if the surface texture is normal and expected or completely
anomalous.

Many thanks,
Nate Chongsiriwatana

Graduate Student
Northwestern University
Department of Chemical and Biological Engineering

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From: vavv2009-at-yahoo.com
Date: Mon, 21 Jan 2008 08:35:15 -0600
Subject: [Microscopy] viaWWW: educational programs, colleges, schools

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Email: vavv2009-at-yahoo.com
Name: Arnold Villanueva

Organization: none

Title-Subject: [Filtered] educational programs, colleges, schools

Question: I am wondering where one can get education (or some type of college degree or certification) to become a Microscopist .. for example, how does one obtain an
associates degree (or certificate or Bachelor's) in Microscopy? any information would be greatly appreciated .. thank you!

Sincerely, Arnold Villanueva

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From: pgan-at-ap.ansell.com
Date: Mon, 21 Jan 2008 08:35:47 -0600
Subject: [Microscopy] viaWWW: ISO 17025 Accreditation on SEM/EDX Analysis

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Email: pgan-at-ap.ansell.com
Name: Gan Phay Fang

Organization: Ansell Shah Alam Sdn Bhd

Title-Subject: [Filtered] ISO 17025 Accreditation on SEM/EDX Analysis

Question: We are thinking of getting an ISO 17025 Accreditation on the SEM/EDX analysis. Our analysis is mostly getting the SEM micrographs and EDX analysis on the polymeric materials. Any advice and comments on starting up the preparation for the ISO 17025 Accreditation are much appreciated.

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From: stephenson-at-impactanalytical.com
Date: Mon, 21 Jan 2008 09:24:01 -0600
Subject: [Microscopy] viaWWW: educational programs, colleges, schools

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Greetings Arnold,

An Associates degree as an electron microscopy technician is available from
the Madison Area Technical College (MATC) in Madison, WI, as well as from
the San Joaquin Delta College of Stockton, CA. Central Michigan University
in Mount Pleasant, MI also has an excellent program that combines an
electron microscopy emphasis with an undergraduate biology degree. These
are the programs that I am aware of.

Yours,
Matthew Stephenson
Impact Analytical/Michigan Molecular Institute


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Email: vavv2009-at-yahoo.com
Name: Arnold Villanueva

Organization: none

Title-Subject: [Filtered] educational programs, colleges, schools

Question: I am wondering where one can get education (or some type of
college degree or certification) to become a Microscopist .. for example,
how does one obtain an
associates degree (or certificate or Bachelor's) in Microscopy? any
information would be greatly appreciated .. thank you!

Sincerely, Arnold Villanueva

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From: smalinskas-at-yahoo.com
Date: Mon, 21 Jan 2008 09:54:49 -0600
Subject: [Microscopy] Re: viaWWW: ISO 17025 Accreditation on SEM/EDX Analysis

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Gan, is accreditation really needed? When our quality
system was staring up and gelling (QS 9000, ISO 17025,
now TS 16949), there was a lot of discussion in our
company early on about how our SEM would fit in. The
end result is that our SEM and EDS are not in our
company's quality system. It is more of a diagnostic
tool and it doesn't factor in to the production of our
product (bearings). Our unit has a sticker on it that
says "Not for product conformance".

Face it, The SEM is just an imaging device like a
fancy camera. Are your cameras in the quality
system?... probably not. Some people think because
they have a highly expensive and technical piece of
equipment, that it needs to be in the quality system.
If you're measuring something, then this issue merits
consideration.

As far as EDS analysis goes, I report semiquantitative
results without numbers. My results are described in
words, because numbers imply accuracy, and any quality
auditor (or client) will want to know the error limits
of reported numbers.

Stu Smalinskas, P.E.
SKF North American Technical Center
Plymouth, Michigan
(734) 414-6862

--- pgan-at-ap.ansell.com wrote:
} Email: pgan-at-ap.ansell.com
} Name: Gan Phay Fang
}
} Organization: Ansell Shah Alam Sdn Bhd
}
} Title-Subject: [Filtered] ISO 17025 Accreditation on
} SEM/EDX Analysis
}
} Question: We are thinking of getting an ISO 17025
} Accreditation on the SEM/EDX analysis. Our analysis
} is mostly getting the SEM micrographs and EDX
} analysis on the polymeric materials. Any advice and
} comments on starting up the preparation for the ISO
} 17025 Accreditation are much appreciated.
}
}


____________________________________________________________________________________
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From: beaurega-at-westol.com
Date: Mon, 21 Jan 2008 11:22:28 -0600
Subject: [Microscopy] RE: Product for watercooling

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi,

FEI servicemen recommend using only distilled or deionized (DI) water in
chilled water recirculator systems.

A very effective algae killer is a long chain quaternary ammonium salt
surfactant that you can buy at any quality swimming pool dealer. IMO,
these quat's are much much better at killing algae than adding available
chlorine from whatever chlorine source. The dosage rate for the very long
chained surfactant is something like one quart per 10,000 gallon of water.
That works out to a low PPM level of a biocide surfactant. Adding a
chlorine-based chemical generates soluble chloride ions that can damage and
can pit corrode stainless steel in DP tubing or SS fittings with O-ring
channels.

There is another side to all this but this next side is rarely discussed.
Algae problems are always discussed on the list server.

If you are running pure DI water, then how can your microscope ever plug up
from green scale? On July 30, 2007 I emailed my FEI serviceman with 25-30
years of microscope experience with Philips-FEI and asked about algae and
scaling. He emailed me the answers. No microscopes that they were asked
to unplug were ever plugged up from algae. It was always green scale that
caused the plugging and the scale was removed with a weak organic acid.

Here are the two sides of the chiller water problem in equation form.

This is the standard belief of the cause of green chiller water and is
shown below as a simplified photosynthesis equation. Quat's efficiently
interrupt the algae cycle on the left-hand side of the equation by breaking
open algae cell walls and killing them. So they never really have a chance
to multiply in a properly run system. Dissociated hypochlorous acid (HClO)
from any chlorine source kills them too but generates additional chloride
ions.

Sunlight + CO2 + H2O + algae ------} O2 + carbohydrates + algae (1)

However, this reaction below is the one that will plug up your microscope
with green scale over time.

2Cu°(s) + H2O + CO2(g) + O2(g) ----} CuCO3(s)oCu(OH)2 green (2)

Notice that CO2 is involved in both reactions. Killing or preventing algae
with a surfactant, an available chlorine oxidizer (hypochlorous acid), or
stopping sunlight will eventually stop the first reaction. Stopping
reaction one only shifts the chemistry focus to reaction two. The problem
is that large stirred chiller systems dissolve more O2 and CO2 at higher
rates than smaller chilled water systems, in my experience. These gases
are dissolved in the pure DI water from the stirring and/or air exposure by
the chiller's unsealed and open reservoir tank of water. Reaction two is
slow and is normally unnoticed until the microscope plugs up. It takes
awhile to notice the copper ion build up unless you regularly test the
chilled water for PPM levels of copper by AA spectroscopy to determine the
rate of copper ion buildup. Furthermore, short light paths of one to three
centimeters or looking through a 6 mm piece of transparent tubing is just
not that effective in spotting the first stages of soluble copper ion build
up by trying to detect a faint initial green color.

I could say much more about the mechanisms, the effect of copper surface
area of exposure, scale distribution in pipes, mechanical devices to add,
and how the Ksp of copper carbonate enters into all this. Here are simple
tests and hints to sort out the situation.

1. Test One. Adding a quaternary ammonium salt surfactant to green water
will kill algae in about an hour. You can use excessive hypochlorite ion
(bleach) on a chiller water sample also. A loss of green color means that
a lot of algae were present.
2. Test Two. Adding ammonium hydroxide to a sample of green chiller water
will turn any dissolved PPM levels of copper ions dark blue at a very high
pH. A positive dark blue copper complex color means that soluble copper
ions are being formed and those ions are tinting the water green.
3. BOTH of these two tests should be done to sort out what your system is
doing.
4. PPM levels of copper ions will kill algae.
5. So you should either have a green algae problem or you have a green
dissolved copper ion problem.
When the copper ions build up in solution from the continuous dissolution
of CO2 and O2, they will exceed the copper carbonate Ksp and start to
precipitate the carbonate to form the green basic copper carbonate scale
shown above.
6. In order to prevent scale formation, you MUST periodically drain out
25%-50% of the chiller water every 3-6 months. This draining and refilling
action is another way to prevent the copper ions and carbonate ions from
exceeding the Ksp value of copper carbonate, which has a lower Ksp than
CaCO3.
7. If forced to use city water, you should flush out the "hard" city water
in instrument dead volumes with DI water to help avoid any mixed carbonate
scaling involving Ca and Mg.
8. Items 6 & 7 almost make an automatic DI water refill system at the
reservoir tank mandatory in large systems. It only has to run when you
will be flushing, refilling, or performing some other planned loss of
chilled water.

Disclaimer: The way additional mechanical features and the chemistry
interact can vary a lot in a custom installed central system and with the
various needs of differnet user's instruments. It is important that users
of central chilled water recirculators understand how their actions, such
as flushing with city water, can have an impact on other users.
IMO, this training is absolutely necessary for users and needed to make
facility engineers understand why certain devices added to a central system
are needed.
This carbonate is the green corrosion product that slowly forms on copper
roofs and gutters from only air and water exposure. The first thin brown
scale color on copper roofs and in pipes is black to dark-brown copper
oxide (CuO). After that forms and with further CO2 exposure, reaction two
is followed.

HTH,

Paul Beauregard
Senior Research Associate, retired
Greensburg, PA
724-834-2247


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From: heller-at-uni-hohenheim.de
Date: Mon, 21 Jan 2008 14:44:02 -0600
Subject: [Microscopy] sectioning watermelon seeds

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Dear Beth,

I only have experience in sectioning seeds of Orobanche cumana. I was
successful doing semi- and ultrathin sections after embedding in LR-White. The
first prepartion step was to perforate the seeds with a fine needle. Without
perforating the seed coat, it was impossible to get anything into these tiny
seeds.

I think seeds are always diffcult, because their coat is quite tight, their
water content extremely low, and they store masses of starch grains or other
storage material which are difficult to fix and to section. Watermelon seeds
are quite large. Maybe you can cut them and try to embed the pieces?

Good Luck,
Anne

} ----------------------------------------------------------------------------
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of America
} To Subscribe/Unsubscribe -- http://www.microscopy.com/MicroscopyListserver
} On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} ----------------------------------------------------------------------------
}
} Hi all,
} Happy New Year!
} Does anyone have experience thick-sectioning watermelon seeds? We're
} working with mature seeds - black seed coat - unfixed, not embedded.
} The seeds are left in a moist chamber overnight to imbibe water.
} Vibratome sectioning didn't work well. Any suggestions? Would fixing
} and embedding make them easier to section?
}
} I think they're really only good for spitting...but the researcher
} doesn't want to hear that;-)
} Any help would be greatly appreciated.
} Many thanks,
} Beth
}
} Beth Richardson
} Plant Biology Department
} University of Georgia
} Athens, GA 30602
} 706-542-1790
}
}
} ==============================Original Headers==============================
} 4, 19 -- From beth-at-plantbio.uga.edu Thu Jan 17 10:21:22 2008
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} 4, 19 -- From: Beth Richardson {beth-at-plantbio.uga.edu}
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}



==============================Original Headers==============================
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7, 32 -- From: heller-at-uni-hohenheim.de
7, 32 -- To: Microscopy-at-microscopy.com
7, 32 -- Subject: sectioning watermelon seeds
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From: nizets2-at-yahoo.com
Date: Tue, 22 Jan 2008 06:29:58 -0600
Subject: [Microscopy] sectioning watermelon seeds

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi!

I am not specialist in botanics, but my common sense tells me that perhaps you could cut the seed in 2 in the length, it would (1) make it thin enough for the fixative to efficiently penetrate (2) avoid the need to perforate the coat. If it is still too thick (for example the tissue next to the coat has artifacts), you could perhaps cut slices.

Regards,

Stephane


----- Original Message ----
X-from: "heller-at-uni-hohenheim.de" {heller-at-uni-hohenheim.de}
To: nizets2-at-yahoo.com
Sent: Monday, January 21, 2008 9:49:20 PM

Dear Beth,

I only have experience in sectioning seeds of Orobanche cumana. I was
successful doing semi- and ultrathin sections after embedding in LR-White. The
first prepartion step was to perforate the seeds with a fine needle. Without
perforating the seed coat, it was impossible to get anything into these tiny
seeds.

I think seeds are always diffcult, because their coat is quite tight, their
water content extremely low, and they store masses of starch grains or other
storage material which are difficult to fix and to section. Watermelon seeds
are quite large. Maybe you can cut them and try to embed the pieces?

Good Luck,
Anne

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} Hi all,
} Happy New Year!
} Does anyone have experience thick-sectioning watermelon seeds? We're
} working with mature seeds - black seed coat - unfixed, not embedded.
} The seeds are left in a moist chamber overnight to imbibe water.
} Vibratome sectioning didn't work well. Any suggestions? Would fixing
} and embedding make them easier to section?
}
} I think they're really only good for spitting...but the researcher
} doesn't want to hear that;-)
} Any help would be greatly appreciated.
} Many thanks,
} Beth
}
} Beth Richardson
} Plant Biology Department
} University of Georgia
} Athens, GA 30602
} 706-542-1790
}
}
} ==============================Original Headers==============================
} 4, 19 -- From beth-at-plantbio.uga.edu Thu Jan 17 10:21:22 2008
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____________________________________________________________________________________
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20, 20 -- From: Stephane Nizet {nizets2-at-yahoo.com}
20, 20 -- Subject: Re: [Microscopy] sectioning watermelon seeds
20, 20 -- To: heller-at-uni-hohenheim.de
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From: quinntl-at-umkc.edu
Date: Tue, 22 Jan 2008 09:00:26 -0600
Subject: [Microscopy] viaWWW: Freeze fracture cell culture

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Email: quinntl-at-umkc.edu
Name: Tim

Organization: UMKC Medical School

Title-Subject: [Filtered] Freeze fracture cell culture

Question: Hello Listies,

I would like to try to freeze fracture cell cultures to look at morphology when exposed to a toxicant.

I don't have special equipment. I practiced a method in school using the ototo protocol in liquid nitrogen but I've lost the protocol.

If anyone has a protocol for freeze fracture on cell culture without utilizing special equipment please reply.

Cheers,

Tim Quinn
UMKC MED SCHOOL
quinntl-at-umkc.edu

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11, 11 -- From zaluzec-at-microscopy.com Tue Jan 22 09:00:26 2008
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11, 11 -- Subject: viaWWW: Freeze fracture cell culture
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From: susan.trant-at-viha.ca
Date: Tue, 22 Jan 2008 09:01:36 -0600
Subject: [Microscopy] viaWWW: Jeol 100CX-II Available

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Email: susan.trant-at-viha.ca
Name: Susan Trant

Organization: Vancouver Island Health Authority

Title-Subject: [Filtered] Jeol 100CX-II

Question: Hello Everyone

We have purchased a new Jeol TEM microscope. We are asking anyone out there if they would like our old Jeol 100CX-II. The vendors have told us that they will crate the microscope up and then it is ours to dispose of. The lucky party must pay to have the microscope shipped to their location.

Sue Trant
EM Technologist
Vancouver Island Health Authority
1952 Bay Street
Victoria BC
V8R 1J8
250-370-8402

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8, 11 -- From zaluzec-at-microscopy.com Tue Jan 22 09:01:35 2008
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8, 11 -- Subject: viaWWW: Jeol 100CX-II Available
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From: hullberg-at-mccrone.com
Date: Tue, 22 Jan 2008 09:04:08 -0600
Subject: [Microscopy] viaWWW: Project MICRO: New Sandbox Contact

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Email: hullberg-at-mccrone.com
Name: Heidi Ullberg

Organization: McCrone Associates, Inc.

Title-Subject: [Filtered] Project MICRO: New Sandbox Contact

Question: We are pleased to announce that the Microscopy Society of Americaís (MSA) collection of sand for use with Project MICRO Microscopic Explorations activity 6 is now housed at McCrone Associates, Inc. in Westmont , Illinois; and is under the direction of Heidi Ullberg.
Mr. Joe Neilly has faithfully dispatched sand samples to educators all over the country for many years. Joe has enjoyed his duties as ëKeeper of the Sandboxí, and as he passes the shovel to Heidi says that he will miss visiting the far reaches of the world - one sand sample at a time.

To view an inventory of the collection visit MSAís website at:

http://microscopy.org/ProjectMicro/Sand/SandCollection.html

To request sand samples, for educational purposes only, please email your request to hullberg-at-mccrone.com .

Please consider donating sand samples to help keep the SANDBOX full. Donations can be mailed to:

SANDBOX
Heidi Ullberg
McCrone Associates, Inc.
850 Pasquinelli Drive
Westmont, Illinois 60559-5539


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From: holsen-at-awscorp.com
Date: Tue, 22 Jan 2008 23:08:58 -0600
Subject: [Microscopy] viaWWW: vacuum pump applications to SEM

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Email: holsen-at-awscorp.com
Name: Harald Olsen

Organization: American World Services

Title-Subject: [Filtered] vacuum pump applications to SEM

Question: Hello,

I work at American World Services in Washington, D.C., we represent the French vacuum pump company Normetex. I was referred to this listserv by Jon Norenburg of the American Microscopical Society as a way to get an answer to a question I have concerning and application for a specific type of ultrahigh vacuum pump.

I have heard that SEM and TEM rely on vacuum pumps, I am trying to figure out if they are similar to the product we represent. Normetex's pumps have traditionally been used in nuclear applications, as they are perfectly clean and dry and thus suited to a clean room environment. Because of their ability to safely handle corrosive or inert gases, I was wondering if they might also have an application with electron microscopy.

In terms of specifications, Normetex produces pumps that range in size from 15 m3/h to 600 m3/h, and produce an ultimate vacuum of 45 mbar on smaller models and 8x10-2 mbar on the larger models.

I am trying to figure out if these pumps would be appropriate for SEM or TEM, as well as who might best be able to make use of them. I realize that this is a very specific question, but I trust that if any resource would have an answer, it would be the members of this listserv.

Thank you,

Harald Olsen
Project Assistant
American World Services Corp.
1247 Wisconsin Ave., NW, Suite 201
Washington, DC 20007
(t) +1.202.296.3523
(f) +1.202.333.0017
holsen-at-awscorp.com
www.awscorp.com


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From: edelmare-at-muohio.edu
Date: Wed, 23 Jan 2008 07:23:02 -0600
Subject: [Microscopy] Refurbishing - Updating Water chillers

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Has anyone on the list had any experiences (Good or Bad) updating the
refrigeration system on a water chiller from R-12 to a current
refrigerant (i.e. R-134a, etc.)?

We have had a older R-12 Haskris chiller die, and are looking at the
possibility of replacing the compressor and condenser (water cooled),
blowing and flushing out the lines, and refilling with a current R-12
replacement. The question is the mineral oil in the system. The R-
12 will replace easily, but what about the residual mineral oil.

Five years ago we updated a chiller, replacing the condenser and
compressor, but we used synthetic oil (instead of mineral oil)
however we still had R-12 so that´s what we used. The system has run
perfectly fine 24/7 for 5 years. This would seem to say oil
incompatibility is not a significant issue.

O.k., I´m being cheap. If I had $6000 I´d buy a new water chiller
and be done with it. But I don´t. I´m hoping for a lower cost
solution that will get me some time. Any thoughts?

Yes, we have professional refrigeration folks working on it but they
are not sure on the smaller systems.

(Disclaimer: I have no financial interests in any refrigeration
company, and have been working with Haskris systems for 25 years and
love them.)


Richard E. Edelmann, Ph.D.
Electron Microscopy Facility Director
364 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



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From: kraftpiano-at-gmail.com
Date: Wed, 23 Jan 2008 09:46:10 -0600
Subject: [Microscopy] Manual for a Consolidated Electrodynamics Corp. type 2201-03 Vacuum gauge.

Contents Retrieved from Microscopy Listserver Archives
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Does anyone have any documentation for a Consolidated Electrodynamics
type 2201-03 Pirani gauge?

Thanks,

Justin A. Kraft

==============================Original Headers==============================
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3, 27 -- Date: Wed, 23 Jan 2008 10:46:08 -0500
3, 27 -- From: "Justin Kraft" {kraftpiano-at-gmail.com}
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From: mbrown-at-aaechighschools.com
Date: Wed, 23 Jan 2008 13:05:04 -0600
Subject: [Microscopy] Issues with a Cambridge S200 SEM

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Our highschool has a Cambridge S200 SEM that was donated to us by
Motorola. They actually donated two, and after months of assembling the
most trustworthy pieces together as one unit, the thing now powers up,
the pumps work and the screen lights up. All I can see on the screen is
snow. No moving of apertures, stage or console controls seem to affect
what is seen on the screen or produces an image. I am reasonably sure
that the Wallace unit is putting out all the high voltages, so the
detector should be getting power. The detector was removed from the
scope and tested with a light, and it does produce a signal under these
circumstances. Connected back to the column though, I see no signal on
my oscilloscope at the test point on the input board for the signal from
the detector, suggesting it is not doing anything. Feeding a test signal
into the microscope at this same test point, I can visualize the signal
on the screen, so the video electronics are working.

The filament fail light goes out when I turn up the filament, so I
assume electrons should be speedng down the column and hitting the
specimen. To the best of my ability the filament is centered and aligned
in the cap properly.

This seems to be the only remaining issue with the microscope, after
solving numerous others, but it has me stumped. The detector apparantly
works, but it isn't working! Any advice?


-Dr. Mike Brown
Science Dept Chair
AAEC_PV




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From: mlibbee-at-gmail.com
Date: Wed, 23 Jan 2008 15:18:22 -0600
Subject: [Microscopy] viaWWW: Allied Epoxy Bond 110

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Email: mlibbee-at-gmail.com
Name: Marissa

Title-Subject: [Filtered] Allied Epoxy Bond 110

Question: I recently found Allied's 2-part Epoxy Bond 110 in my lab but could not locate the mixing literature. I've emailed Allied but am rather impatient...Does anyone know the ratio of resin to hardener and the temperature necessary to cure the epoxy?

Thank you!

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From: swaffordisjim-at-gmail.com
Date: Wed, 23 Jan 2008 15:18:49 -0600
Subject: [Microscopy] viaWWW: MT1 Ultra microtome

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Email: swaffordisjim-at-gmail.com
Name: Jim Swafford

Organization: retired on Dinjim ranch

Title-Subject: [Filtered] MT1 Ultra microtome

Question: Greetings.
I am wanting to purchase a particular model of ultra microtome, Sorvall MT1, which was very popular in the late 1950's through 1960's. I anticipate using this instrument at Pittsburg State University which is a small school,
~6,000 students, located in Southeastern Kansas.
If anyone knows the location of one of these microtomes that could be sold or donated, please contact me.

Thanks very much. Jim

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From: connellyps-at-nhlbi.nih.gov
Date: Wed, 23 Jan 2008 17:57:24 -0600
Subject: [Microscopy] Interest in smaller "Permanox" dishes?

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Greetings,

For quite some time I have wondered why NUNC did not make a Permanox Petri
Dish smaller than 60 x 15 mm. I have grown to really appreciate the
advantages of using the Permanox over standard Polystyrene dishes for tissue
cultured cells grown for TEM experiments since every cell line that I have
tried adheres well to them, they can withstand chemicals like acetone and
propylene oxide that dissolve the polystyrene and the embedded cells come
away from the Permanox so easily and smoothly.

With the special cells and reagents that I am now using for TEM, it is a big
waste to grow cells over such a large area when a 35 x 15 mm dish would do
nicely. I do want a dish not a chambered slide.

I would like to know if there are others (you)
1. who would switch to a smaller dish if they would be made available.
(this is my pick)
2. who would like to use both the 60mm and 35mm dishes
3. who would only use the 60mm dishes
If I get a reasonable response I will contact the company with my results to
back up my request that they consider making the smaller dishes.

Comments are welcome.

For the survey, it may be best to answer me "Off-ListServer" so as not to
fill up the emails of other members. I will let the ListServer know the
tally after the replies come in.

Thanks to all,
Pat

Patricia Stranen Connelly
Biologist, Electron Microscopy
NHLBI Electron Microscopy Core
National Institutes of Health
14 Service Road South
Bldg. 14E ­ Rm. 111B MSC 5570
Bethesda, MD 20892-5570
Phone 301-496-3491
FAX 301-480-6560
connellyps-at-mail.nih.gov



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From: david.knecht-at-uconn.edu
Date: Thu, 24 Jan 2008 08:19:42 -0600
Subject: [Microscopy] Infinity corrected objectives

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

I have a user who was trying to use a camera without microscope to
image something that he could not get on the stage of the microscope.
In playing around, he discovered that Nikon objectives actually have a
C-mount compatible thread. When he screwed a 2cm extender and then a
20x objective onto the CCD camera, he was able to image a specimen at
a distance of about 2cm. Naively, I would have said that an infinity
corrected lens should not form an image in the plane of the CCD chip,
but obviously, the specimen is not at the appropriate focal point of
the lens (~2mm). Can someone explain why this works? Thanks- Dave

Dr. David Knecht
Department of Molecular and Cell Biology
Co-head Flow Cytometry and Confocal Microscopy Facility
U-3125
91 N. Eagleville Rd.
University of Connecticut
Storrs, CT 06269
860-486-2200
860-486-4331 (fax)



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From: kenconverse-at-qualityimages.biz
Date: Thu, 24 Jan 2008 10:29:16 -0600
Subject: [Microscopy] Issues with a Cambridge S200 SEM

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Mike,
Are you getting emission current? Does it (emission current) appear to
behave properly as you heat the filament? If not, then there is some kind
of problem with the gun circuit. If so, I'd say the beam isn't making it
down the column. Are the various beam-steering circuits behaving properly?
Have you tried pulling out all the apertures to try and get some response?
Are both the upper and lower scan coils functioning properly? Any of the
coils have the potential to drive the beam off to the side somewhere and
make it disappear.

Ken Converse
owner

QUALITY IMAGES
Servicing Scanning Electron Microscopes
Since 1981
474 So. Bridgton Rd.
Bridgton, ME 04009
207-647-4348
Fax 207-647-2688
kenconverse-at-qualityimages.biz
qualityimages.biz



-----Original Message-----
X-from: mbrown-at-aaechighschools.com [mailto:mbrown-at-aaechighschools.com]
Sent: Wednesday, January 23, 2008 2:08 PM
To: kenconverse-at-qualityimages.biz

Our highschool has a Cambridge S200 SEM that was donated to us by Motorola.
They actually donated two, and after months of assembling the most
trustworthy pieces together as one unit, the thing now powers up, the pumps
work and the screen lights up. All I can see on the screen is snow. No
moving of apertures, stage or console controls seem to affect what is seen
on the screen or produces an image. I am reasonably sure that the Wallace
unit is putting out all the high voltages, so the detector should be getting
power. The detector was removed from the scope and tested with a light, and
it does produce a signal under these circumstances. Connected back to the
column though, I see no signal on my oscilloscope at the test point on the
input board for the signal from the detector, suggesting it is not doing
anything. Feeding a test signal into the microscope at this same test point,
I can visualize the signal on the screen, so the video electronics are
working.

The filament fail light goes out when I turn up the filament, so I assume
electrons should be speedng down the column and hitting the specimen. To the
best of my ability the filament is centered and aligned in the cap properly.

This seems to be the only remaining issue with the microscope, after solving
numerous others, but it has me stumped. The detector apparantly works, but
it isn't working! Any advice?


-Dr. Mike Brown
Science Dept Chair
AAEC_PV




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From: cervantes-at-bendres.com
Date: Thu, 24 Jan 2008 10:53:48 -0600
Subject: [Microscopy] ESEM Imaging of Live Cells

Contents Retrieved from Microscopy Listserver Archives
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Hi All -
I would appreciate hearing from users of environmental SEMs, specifically as to imaging live cells. This is a new area for me, as my expertise is in TEM, so I am trying to gather as much information as possible.

We already have a variable pressure SEM, which is not ideal for viewing cells, although to my knowledge we have never tried it. I have been looking at manufacturers of ESEMs, and have found the Zeiss EVO LS and the FEI Quanta. Any user opinions on these two systems are welcome as well.

Thanks,
Jessica
____________________
Jessica Cervantes
Bend Research Inc
Bend, OR 97701
www.bendres.com

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From: bfostermme-at-sbcglobal.net
Date: Thu, 24 Jan 2008 13:17:30 -0600
Subject: [Microscopy] Re: Infinity corrected objectives

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi, David

Clever set up!

The answer is quite simple. For the sake of simplicity, a compound microscope has two key "imaging" lenses: the objective and the eyepiece. Optically, the job of the eyepiece is to create a (usually) magnified image at the appropriate location to act as a "specimen" for the eyepiece. In order for there to be an image, the light carrying the original specimen information must convege to a point of focus. There are two ways to achieve that result:
a. To place the object just beyond the front focal plane of the objective (FFPo), resulting in a real image at some fixed distance
b. To place the object exactly at the FFPo, sending the imaging information up through the optical train in a bundle of rays which is either parallel to the optic axis (on-axis info) or some principle ray at some angle to that axis (off-axis info). Note that if these rays are parallel, they cannot converge to form an image. We say that the information "goes to inifinity", hence never forms an image. In this case, you need a second lens (the telan or tube lense) to create the necessary convergence at the right location for the eyepiece. The space between the back focal plane of the objective and the tube lens is what is known as infinity space, a design which gives considerable freedom to microscope designers.

So, if you take a lens that was meant to work in Condition b and move the object slightly further away from the front of the lens, you will change the optics to Condition a. This is another one of those cases, like NA, where what is written on the objective is only true when the microscope is properly set up and aligned for Koehler illumination.

Hope this was helpful!

Best regards,
Barbara Foster, President

Microscopy/Microscopy Education
7101 Royal Glen Trail, Suite A
McKinney TX 75070
P: (972)924-5310
Skype: fostermme
W: www.MicroscopyEducation.com


MME is now scheduling customized, on-site courses through July 2008. Call us today for details.

We are sorry to report that Optimizing Light Microscopy for the Biological and Clinical Laboratory is no longer available.



At 08:34 AM 1/24/2008, you wrote:



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From: mbrown-at-aaechighschools.com
Date: Thu, 24 Jan 2008 14:33:50 -0600
Subject: [Microscopy] Latest on the Cambridge S200 with no image

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Thank you to the dozens of you who sent in suggestions. Most
suggestions were that electrons were not making it down the column to
the specimen. I removed one of the apertures. Electrons are now
getting down the column to the specimen when I dial in the place where
the aperture used to be. When I turn up the filament until the fail
light goes off, the screen flashes, and the nature of the snow on the
screen changes. I can visualize vertical stripes down the screen.
These move around to the left and right when I move the specimen.
Rotating the image moves the lines also, but they always stay vertical.
In fact rotating the specimen also moves the vertical lines but does not
make them horizontal.

What is the issue here?

-Dr. Mike Brown
Science Dept Chair
AAEC_PV




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From: stephen.ruiz-at-siemens.com
Date: Thu, 24 Jan 2008 18:24:26 -0600
Subject: [Microscopy] AskAMicroscopist: Digital SLR Camera

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This Question was submitted to Ask-A-Microscopist by (stephen.ruiz-at-siemens.com)
from http://www.microscopy.org/Ask-A-Microscopist/Ask-A-Microscopist.html on Thursday, January 24, 2008 at 14:41:03
Remember to consider the Grade/Age of the student when considering the Question
---------------------------------------------------------------------------
Please reply to both stephen.ruiz-at-siemens.com as well as to the Microscopy Listserver
---------------------------------------------------------------------------

Email: stephen.ruiz-at-siemens.com
Name: Stephen Ruiz

Organization: Siemens DX

Education: Graduate College

Location: Norwood, Ma., USA

Title: Digital SLR Camera

Question: Any suggestions on a good SLR digital camera for both micro and macro images?

---------------------------------------------------------------------------

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From: bfostermme-at-sbcglobal.net
Date: Thu, 24 Jan 2008 18:45:14 -0600
Subject: [Microscopy] Infinity corrected objectives - some

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Dear Listers,

David sent me a follow-up to this posting, asking how to incorporate all of this info into teaching microscopy. I know that a number of you teach and might find the infomration useful, so here's a copy of my answer to him.

Dear David,

There is a really neat way to do all of this. It starts with a simple experiment with a hand lens.
a. Difference between object and image
Using a simple hand lens, have the students look through the lens at their finger nails (be prepared for lots of silly groans!). First have them put their finger close to the lens, then have them slowly move it back. As they do, the image of their finger will become larger and larger. At some point it will disappear. Then, if they keep watching carefully, the image will reappear, inverted.
Then, have them remove the lens and look directly at their finger. At this point I tell the, "Notice that at no point did your finger leave your hand." This really solidifies the concept of object (their finger) and image (what they saw through the lens, after the lens has operated on that information. Take home message: our job as microscopists is to capture in the image, with as much fidelity as possible, the information from the object. Second take home messages: Lenses can lie.

b. Find the focal length of the lens
Using a simple, single hand lens, have the students find the focus the image of the overhead lights on the table in front of them. The distance from the physical center of the lens to the table top is the focal length. This set up the following concepts:
Focal length
Focal plane
Front focal plane

c. Four cases of lens
Now that they understand the concept of object/image and focal length, you can repeat Experiment A to illustrate the case of the object
(1) inside the focal length (forms virtual, upright image on same side of the lens as the object
(2) at the focal length (informrtion goes to infinity: no convergence of date; No image)
(3) slightly beyond the focal length (real image, on other side of the lens; magnification determined by distance of object from lens)
(4) a great distance beyond the focal length (light coming from "infinity"; rays form bundle which is parallel to either optic axis or principle ray through optical axis).
You can reinforce all of these using simple ray diagrams found in any high school physics book.

d. All of this sets up the discussion for
(1) Infinity vs. fixed tube length optics and why you just can't willy nilly change objectives from stands of one design to stands of the other
(2) Spherical and chromatic aberration
(3) Which then leads to discussions of different types of glassware on the microscope and how to make educated buying decisions based on corrections, working distances.

It's a great set of lecture/demonstrations that really carries through to discussions of NA, resolution versus detection, and contrast techniques...a little bit of physics that goes a long way. And because they are doing demonstrations throughout the lecture, they stay involved AND tend to remember it all (every teachers' dream).

At this point, I'd recommend getting a copy of my book... it's all in there... but we have just come to the end of the supply. I need to talk to Zeiss, to see if they are interested in updating and reprinting. My other challenge is finding the time to do that. I do have some lecture notes that I use when I teach, but they are primarily just the diagrams, etc.

Hope this was helpful.

Best regards,
Barbara




At 04:11 PM 1/24/2008, you wrote:
} THanks for the explanation. It makes sense and the object(ive) lesson is especially important (abberations aside). I will have to think how I can incorporate this into my microscopy course. Dave
}
} On Jan 24, 2008, at 2:17 PM, {mailto:bfostermme-at-sbcglobal.net} bfostermme-at-sbcglobal.net wrote:
}
} }
} }
} }
} } ----------------------------------------------------------------------------
} } The Microscopy ListServer -- CoSponsor: The Microscopy Society of America



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From: maloneyb-at-fiu.edu
Date: Fri, 25 Jan 2008 05:14:12 -0600
Subject: [Microscopy] digital camera with lens vs. fiber optic coupled camera

Contents Retrieved from Microscopy Listserver Archives
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Dear Group - what is your opinion for a TEM bottom mounted camera for
the best resolution for high mag - camera with lens or fiber optic?
Appreciate any comments.
Thanks
Barbara

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From: reinhard.rachel-at-biologie.uni-regensburg.de
Date: Fri, 25 Jan 2008 07:23:23 -0600
Subject: [Microscopy] digital camera

Contents Retrieved from Microscopy Listserver Archives
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} TEM bottom mounted camera for high res imaging:

only fiber optic coupling - as far as I can tell.
best regards
Reinhard Rachel
--

----------------------
PD Dr. Reinhard Rachel
Universitaet Regensburg
Centre for EM - NWF III -
-at-Institute for Anatomy
Universitaetsstr. 31
D-93053 Regensburg - Germany
tel +49 941 943 2837, 1720
fax +49 941 943 2868
mail reinhard.rachel-at-biologie.uni-r.de
office: VKL 3.1.29



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From: mike-at-bitplane.com
Date: Fri, 25 Jan 2008 09:11:08 -0600
Subject: [Microscopy] Job Posting

Contents Retrieved from Microscopy Listserver Archives
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Sales and Sales Support Positions Available in the USA

Position #1 – Central and South Eastern Region Sales Representative US /
Canada

Bitplane is looking for a biologist with strong computer skills and at least
one year of hands-on experience using a confocal or similar 3D advanced
light microscope.

Feel free to forward this e-mail if know someone in your facility who would
be interested.

The duties of this position include:

• Customer visits and analysis of customer's imaging needs.
• Demonstration of the software and onsite work with the customer
• Organization of exhibitions and workshops.
• Sales support of existing customers.
The candidate is expected to have an outgoing personality with strong
communication skills and should look forward to increased responsibility. At
least 50% travel will be required.  Representative is required to live in
the territory they cover.  Benefits include a base salary, performance based
commission, 401K plan, healthcare, and vacation.  Representative will work
out of a home office. We offer a team of 18 people, fun to work with, and a
truly international environment that provides the resources required to
grow. We don't mind if the candidate does not have much business experience
and we are prepared to show him/her the sales skills at the job.

Position #2 – Sales Support Manager

Bitplane is looking for a candidate with a science background and knowledge
of the confocal and 3D microscope community. 

Feel free to forward this e-mail if know someone in your facility who would
be interested.

The duties of this position include:

• Identifying potential new regional customers via web searches, literature
searches, marketing campaigns, trade shows, and customer referrals.
• Introduction of Bitplane products and services to potential customers via
email, phone, and Webex.
• Understanding potential customers needs related to products offered by
Bitplane.
• Organizing and planning workshops and demonstrations for regional sales
representatives

The candidate is expected to have an outgoing personality with strong
communication skills and should look forward to increased responsibility. 
Travel not required.  Benefits include a base salary, 401K plan, healthcare,
and vacation.  Representative will work out of a home office. We offer a
team of 18 people, fun to work with, and a truly international environment
that provides the resources required to grow.

Bitplane is an international company specializing in the sale of software
for the visualization and analysis of 3D and 4D microscope images.  More
information can be found at www.bitplane.com

Interested persons should respond directly to Michael C. Wussow
(mike-at-bitplane.com 651-336-4600) indicating which position they are
interested in and providing a copy of their CV.

Bitplane Inc.
Michael C. Wussow
Vice President and General Manager Bitplane Inc.
 
Cell Phone:    651-336-4600
Fax:                 866-691-9112
Toll Free:       1-888-3D-BITPX (332-4879)
Visit Our Web Site At:  www.bitplane.com





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From: bliss5-at-llnl.gov
Date: Fri, 25 Jan 2008 12:34:53 -0600
Subject: [Microscopy] JEOL 733 problems

Contents Retrieved from Microscopy Listserver Archives
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Hello everybody:

We're having some beam instability problems with our tool. The local
fixit person would like to rule out the high voltage as the cause. He
asked me to find an HV tank to substitute. Is it possible someone has
a tank (or other parts) sitting around, gathering dust?

Perhaps someone has had this problem before. After turning on the
beam, the current drops. It wavers and then comes back only to repeat
after a short time. The time periods are approximate; 20 minutes at
first, and 10 minutes in the repeat cycle. If the beam is turned off
for several minutes while the HV is ramped up, there will be a longer
time period before the current drops again.

TIA,
Annie
--

+++++++++++++++++++++++++++++

R. Ann Bliss, Technologist
Chemistry Materials, Earth and Life Sciences
Materials Science and Technology Division
Lawrence Livermore National Laboratory

_____________________________

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From: andrea-at-ncmir.ucsd.edu
Date: Fri, 25 Jan 2008 16:01:52 -0600
Subject: [Microscopy] viaWWW: problems cutting serial thick sections (above 1-2

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Email: andrea-at-ncmir.ucsd.edu
Name: Andrea Thor

Organization: UCSD

Title-Subject: [Filtered] problems cutting serial thick sections (above 1-2 microns) without getting serious pitting of the blockface

Question: I am having some problems in cutting serial thick sections (above 1-2 microns) without getting serious pitting of the blockface. I heard this is not uncommon when pushing the section thickness to the extreme (such as 3-5 microns). We usually deal with the situation by refacing the block after each thick section, but this of course would make true "serial" sectioning impossible.
The blocks I am working with are either cardic left ventricle or striatal tissue embedded in Durcupan.


If anyone has tried or has a protocol or techniques,
I'd be very grateful to hear about them. It
could save us tons of time and frustration as we develop a new set of protocols.

Thanks very much.

Andrea


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From: davefissell-at-yahoo.com
Date: Sat, 26 Jan 2008 09:46:02 -0600
Subject: [Microscopy] AskAMicroscopist: Microscope Ergonomics

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Email: davefissell-at-yahoo.com
Name: David Fissell

Organization: CSU-DH

Education: Graduate College

Location: Brownsburg, IN, USA

Title: Microscope Ergonomics

Question: Visual inspection with a microscope is a common work situation for many industries. It is believed, poor ergonomic design of workstations where work demands involving a microscope are high (4-6 hours/work day) result in substandard performance. My question: Are you familiar with any research/industry guidelines supporting or countering this believe? Do you know of any ergonomic guidelines/standards prescribed for microscopist workstation design?
Thank You
David
PS: My specific area of research is the impact on visual perception in industrial behavioral situations.

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From: z.zhou-at-sheffield.ac.uk
Date: Mon, 28 Jan 2008 08:02:40 -0600
Subject: [Microscopy] viaWWW:FIB - carbon deposition quality

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http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

David

I am not sure of any specific health and safety regulations issued
by any any safety organizations.

But I would suggest that appropriate or
similar regulations such as would be useful:
1. The provision, use and
maintenance of workplace equipment (PUWER 1998 UK safety regulations)
2.
Display Screen Equipment (computers and similar instruments) regulations
(DSE 2002 UK safety regulations)
3. and specific safety handling
regulations for specimens such as chemical, biological and microbiological
where appropriate in the lab.

I did a quick Google search (see below)
and found a few industry and university websites. They all seem to
consider ergonomics, optimal operation, good maintenance, environment,
work activity patterns and nature of the specimen and any chemicals as
most important. Most users seem to prefer binocular eyepieces with a good
range of easy to use adjustments (eg dioptre correction and interocular
distance.

websites:
http://www.manufacturingtalk.com/news/nik/nik109.html

http://ehs.ucdavis.edu/sftynet/sn-27.cfm

http://www.stanford.edu/dept/EHS/prod/general/ergo/labergo.html

http://www.safety.uwa.edu.au/policies/microscopes


I hope this helps and sorry about all the UK safety references but I'm
sure there will be similar US regulations.

Good luck

Malcolm

Malcolm Haswell
e.m. unit
Chemispec
School of Health, Natural and Social Sciences
Fleming Building
University of Sunderland
Tyne & Wear
SR1 3SD
UK
e-mail: malcolm.haswell-at-sunderland.ac.uk

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Email: z.zhou-at-sheffield.ac.uk
Name: Zoe Zhou

Organization: The University of Sheffield

Title-Subject: [Filtered] FIB

Question: I'm using a FEI quanta 200 3D focused ion beam microscope. I find tricky to control and understand the carbon deposition quality. I wonder what the gas injection process is while doing either C or Pt deposition pads. Is it an electron or ion plasma enhanced chemical vapour deposition process? Can anybody lead me to some related literatures?

Zoe

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From: greggps-at-umich.edu
Date: Mon, 28 Jan 2008 08:07:03 -0600
Subject: [Microscopy] AskAMicroscopist: Microscope Ergonomics

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David,
This particular information is considered more critical in the area of
Patholgy, either in pharmaceutical or hospital settings (or associated
contract work). Some pathologists are expected to spend 40 hours a week
doing nothing but reviewing thousands of microscope slides. It is one
case where ergonomic statistics have definitely been researched
extensively, since improving efficiency by a mere 5% can have quite an
impact.

I personally do not have a source for this information, but a pathology
oriented website probably could help.

Good luck,
~Gregg

Gregg Sobocinski
Imaging Specialist/Microscopist
University of Michigan, MCDB Dept.
Ann Arbor, Michigan
USA


-----Original Message-----
X-from: davefissell-at-yahoo.com [mailto:davefissell-at-yahoo.com]
Sent: Saturday, January 26, 2008 10:57 AM
To: Sobocinski, Gregg

This Question was submitted to Ask-A-Microscopist by
(davefissell-at-yahoo.com)
from
http://www.microscopy.org/Ask-A-Microscopist/Ask-A-Microscopist.html on
Saturday, January 26, 2008 at 04:33:33
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Question
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---
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Microscopy Listserver
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---

Email: davefissell-at-yahoo.com
Name: David Fissell

Organization: CSU-DH

Education: Graduate College

Location: Brownsburg, IN, USA

Title: Microscope Ergonomics

Question: Visual inspection with a microscope is a common work situation
for many industries. It is believed, poor ergonomic design of
workstations where work demands involving a microscope are high (4-6
hours/work day) result in substandard performance. My question: Are you
familiar with any research/industry guidelines supporting or countering
this believe? Do you know of any ergonomic guidelines/standards
prescribed for microscopist workstation design?
Thank You
David
PS: My specific area of research is the impact on visual perception in
industrial behavioral situations.

------------------------------------------------------------------------
---

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From: agata.sena-at-hotmail.com
Date: Mon, 28 Jan 2008 08:17:06 -0600
Subject: [Microscopy] AskAMicroscopist: Si, S, Cu and Zn as contaminant in the EDS

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Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (agata.sena-at-hotmail.com) from http://microscopy.com/Ask-A-Microscopist/Ask-A-Microscopist.html on Monday, January 28, 2008 at 05:24:58
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Email: agata.sena-at-hotmail.com
Name: Agata

Organization: Materials Division

Education: Graduate College

Location: Brazil

Question: Dear all:

I'm characterizing gold tips by SEM/EDS. We are measuring the end of the tips and some of them have a deposit. I observed Si, S, Cu and Zn as contaminant in the EDS spectra of the deposit. The measurements are made on a FEI-Nano Lab and EDAX equipments. I didn't see any carbon. Is it possible thta these impurities be coming from SEM chamber by e-beam exposion?

Thanks for any help.
Best Regards.

Agata

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From: kraftpiano-at-gmail.com
Date: Mon, 28 Jan 2008 08:27:34 -0600
Subject: [Microscopy] Chiller pump and lifting power.

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

I finally got sick of the noise and heat being thrown off by my water
chiller system for the SEM, so I decided to move it to another room.
Before I do this, though, the water lines have to be run up into the
ceiling, over about 20 feet, then down to the microscope again. I've
taken into consideration the connection end and plumbed in a valve
system so I have a cut-off to run water through the chiller and piping
without circulating it through the SEM, but I'm still wondering about
the lifting power of the pump. Does the power required to lift the
water lower the flow rate, or does the drop on the other end create
enough of a siphon effect to cancel out any effects of the lift?

I seem to be able to reason this one out either way, depending on
which outcome I'm looking for...

--Justin A. Kraft

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From: TindallR-at-missouri.edu
Date: Mon, 28 Jan 2008 08:46:08 -0600
Subject: [Microscopy] Chiller pump and lifting power.

Contents Retrieved from Microscopy Listserver Archives
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Justin,

I'm sure the chiller manufacturer can answer this question for you. Our
own experience in doing exactly the same thing was that we were able to
run our (Haskris) chiller lines through the ceiling and move the chiller
two rooms away----about 20 feet as the crow walks---with no problems
whatsoever. However, when we needed that room for a new scope and moved
the chiller again, we went a room too far with that extra 10-odd feet.
The TEM began shutting down its lenses at frequent intervals and our
JEOL engineer quickly figured out that the water flow was reduced to the
point that we were running right at the edge of the water's ability to
cool the lenses. A few degrees and the scope would shut them down. We
were due to install a new TEM anyway, so he tweaked the temperature
settings to allow a slight extra increase in temperature before it shut
down, and we limped over the finish line until the new scope came.

Another caution--- when the lines run overhead be very careful to check
for the development of leaks. Water spraying down on equipment can be
fundamentally different that water puddling on the floor (we've had both
happen and we've been lucky each time). Copper lines have the nasty
tendency to occasionally develop pinhole leaks from being etched
internally by distilled water.

So, yes, problems are possible, but it will be a function of chiller
pumping capacity and distance from the scope. Again, check with the
manufacturer.

Good luck!

Randy

Randy Tindall
Senior EM Specialist
Electron Microscopy Core Facility---We Do Small Well!
W125 Veterinary Medicine
University of Missouri
Columbia, MO 65211
Tel: (573) 882-8304
Fax: (573) 884-2227
Email: tindallr-at-missouri.edu
Web: http://www.emc.missouri.edu
On-line calendar:
http://biotech.rnet.missouri.edu/cgi-bin/Calcium310.pl?Op=Splash&Amount=
Week&NavType=Both&Type=TimePlan


-----Original Message-----
X-from: kraftpiano-at-gmail.com [mailto:kraftpiano-at-gmail.com]
Sent: Monday, January 28, 2008 8:28 AM
To: Tindall, Randy D.

I finally got sick of the noise and heat being thrown off by my water
chiller system for the SEM, so I decided to move it to another room.
Before I do this, though, the water lines have to be run up into the
ceiling, over about 20 feet, then down to the microscope again. I've
taken into consideration the connection end and plumbed in a valve
system so I have a cut-off to run water through the chiller and piping
without circulating it through the SEM, but I'm still wondering about
the lifting power of the pump. Does the power required to lift the
water lower the flow rate, or does the drop on the other end create
enough of a siphon effect to cancel out any effects of the lift?

I seem to be able to reason this one out either way, depending on which
outcome I'm looking for...

--Justin A. Kraft

==============================Original
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From: mbrown-at-aaechighschools.com
Date: Mon, 28 Jan 2008 09:41:59 -0600
Subject: [Microscopy] Cambridge S200 schematics

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Does anyone have the schematics for the joystick controller and/or the
high voltage Wallace unit for this microscope?

-Dr. Mike Brown
Science Dept Chair
AAEC_PV




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From: wesaia-at-iastate.edu
Date: Mon, 28 Jan 2008 09:48:00 -0600
Subject: [Microscopy] Chiller pump and lifting power.

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

X-from a plumbing point of view, your latter comment is correct: if the
inlet and outlet are at the same height as before, there is no extra
consideration from running the hose up and down. If the piping system
were open, the height of the loop would be a factor. If there is a
difference in height between inlet and outlet, that must be taken into
account.

However, the bigger concern in this case is the pressure drop due to the
sheer length of tubing involved. Moving the chiller to another room and
adding 15 to 20 feet just to loop over the wall adds a lot of extra flow
restriction. Extra fittings may also be significant. Chemical engineers
have tables of equivalent tube lengths for the many kinds of fittings. I
have forgotten the details, but each fitting adds a substantial length
(maybe up to a foot) to the effective length of the loop. It is good to
keep them to a minimum.

The pressure drop can be handled by switching to a larger pump or by
switching to a larger size hose. However, neither option is cheap.
Consider it as you make your plans.

Warren Straszheim

-----Original Message-----
X-from: kraftpiano-at-gmail.com [mailto:kraftpiano-at-gmail.com]
Sent: Monday, January 28, 2008 8:28 AM
To: wesaia-at-iastate.edu

I finally got sick of the noise and heat being thrown off by my water
chiller system for the SEM, so I decided to move it to another room.
Before I do this, though, the water lines have to be run up into the
ceiling, over about 20 feet, then down to the microscope again. I've
taken into consideration the connection end and plumbed in a valve
system so I have a cut-off to run water through the chiller and piping
without circulating it through the SEM, but I'm still wondering about
the lifting power of the pump. Does the power required to lift the
water lower the flow rate, or does the drop on the other end create
enough of a siphon effect to cancel out any effects of the lift?

I seem to be able to reason this one out either way, depending on
which outcome I'm looking for...

--Justin A. Kraft



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From: beaurega-at-westol.com
Date: Mon, 28 Jan 2008 12:52:54 -0600
Subject: [Microscopy] Re: Chiller pump and lifting power.

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

David,

Like Malcolm, I know of no ergonomic guidelines that are specific to
microscopy. However, folks in our lab have much experience in the areas of
optical, AFM, SEM, TEM and microtomy. We receive generalized training in
ergonomics at my work. However, I have significant personal experience
with ergo problems and know first-hand how painful and long-lasting the
problems can become.

Ergonomically healthy posture when using a stand-alone optical microscope,
TEM or microtome, i.e. without a computer interface, is relatively
straightforward to achieve.
Good, relaxed posture is important. Ensure that a chair equipped
with arm rests is available that allows each analyst to look through
the oculars without hunching over or straining upward.
Minimizing eye strain is essential for long periods of time at an
optical microscope. Ensure that each analyst knows how to adjust the
binoculars to ones interpupillary distance and focus for each eye.
Try to minimize bright lighting above or around the microscope.
Glare and too-bright ambient lighting can pose problems during
extending work on a microscope or computer.

Unfortunately, interfacing a computer, monitor, keyboard and mouse turns a
relatively ergonomically simple instrument into a nightmare for posture.
Our internal ergo consultants have provided some help although they contend
that computerization of microscopes generates hard-to-resolve problems.
The problem that occurs when one integrates a computer with any type of
microscope is that the microscope and computer, ergonomically benign tools
when used correctly, each become difficult to use. It seems that one may
choose to be comfortable at one or the other but not both. Trade-offs tend
to be the rule. I suggest that one achieve the best ergo-friendly setup
for the tool that is used most frequently. If one tends to spend most of
the time at the microscope and only intermittently work at the computer,
then design the ergonomics of the work area around the scope; the converse
should be applied if the primary tool used during analyses is the computer.

Several key points should be made. Please note that repeated reaching or
twisting means even several times during multiple short sessions at the
scope. Ergo problems tend to be cumulative during a day or even days:
Never repeatedly twist the body to reach a tool. Rather, roll the
chair to the tool and assume good posture. It takes a little longer
but will be worthwhile in the end.
Avoid repeated reaching, i.e. extending ones arm, to perform a task.
This can quickly lead to severe shoulder and neck pain.
Take a short break each half hour on the scope. Spending a couple of
minutes to stretch the hands, shoulders, back and neck can work
wonders.
Finally, be aware of minor aches and pains that didn't seem to be
there before. A hand, thumb, arm, shoulder, back or neck that is
even slightly stiff or sore should be stretched and rested before
continuing extensive work on the scope. Varying the type of work
done during the day can be a big help in minimizing or eliminating
ergo problems.
A set of cold eyes is often useful to recognize problems of which
the individual may not aware.

Several guidelines that we have found helpful in the use of computers
follow:
The computer monitor should be adjustable for each, not most,
microscopist. Set the monitor height such that the top of the
monitor field is an inch or so higher than the persons eyes when
looking straight ahead. Avoid looking up or down at a monitor. I
have found that looking upward at a monitor may cause very
significant issues with the neck and shoulders, sometimes in a very
short period of time.
Like monitors, keyboards and mouse(mouses, mice ?) should be
adjustable for each (not most) microscopist. Avoid reaching or
extending the arms to reach the keyboard or mouse. Adjustable
keyboard articulating trays are very useful. The keyboard and mouse
should be set to neutral posture such that the lower arms are
horizontally orientally and the tops of the hands do not bend up or
down.
Consider using fitting the computer with a trackball in addition to
or instead of a mouse. When selecting a trackball, look for one with
the largest ball available. The ball should be one that is moved
with the fingers and/or hands, not the thumb. I use the Kensington
Expert Mouse (I know that other good trackballs exist). The ball is
about the size of a billiard ball.

Keep in mind that solving and correcting ergo problems in microscopy labs
often requires patience and perseverance.

Best regards,


Disclaimer: The comments and opinions given above are those of the author
alone and do not represent any position of ExxonMobil Chemical Company.

Gary M. Brown
Microscopy Specialist
ExxonMobil Chemical Company
Baytown Technology & Engineering - West
5200 Bayway Drive
Baytown, Texas 77520-2101
phone: 281 834 2387
fax: 281 834 2395
e-mail: Gary.M.Brown-at-ExxonMobil.com

"Our business in life is not to succeed, but to continue to fail in good
spirits." Robert Louis Stevenson



----- Forwarded by Gary M Brown/Baytown/ExxonMobil on 01/28/08 10:11 AM
-----

malcolm.haswel
l-at-sunderland.a
c.uk To
gary.m.brown-at-exxonmobil.com
cc
01/28/08 05:10
AM Subject
[Microscopy] Re: AskAMicroscopist:
Microscope Ergonomics
Please respond
to
malcolm.haswel
l-at-sunderland.a
c.uk











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David

I am not sure of any specific health and safety regulations issued
by any any safety organizations.

But I would suggest that appropriate or
similar regulations such as would be useful:
1. The provision, use and
maintenance of workplace equipment (PUWER 1998 UK safety regulations)
2.
Display Screen Equipment (computers and similar instruments) regulations
(DSE 2002 UK safety regulations)
3. and specific safety handling
regulations for specimens such as chemical, biological and microbiological
where appropriate in the lab.

I did a quick Google search (see below)
and found a few industry and university websites. They all seem to
consider ergonomics, optimal operation, good maintenance, environment,
work activity patterns and nature of the specimen and any chemicals as
most important. Most users seem to prefer binocular eyepieces with a good
range of easy to use adjustments (eg dioptre correction and interocular
distance.

websites:
http://www.manufacturingtalk.com/news/nik/nik109.html

http://ehs.ucdavis.edu/sftynet/sn-27.cfm

http://www.stanford.edu/dept/EHS/prod/general/ergo/labergo.html

http://www.safety.uwa.edu.au/policies/microscopes


I hope this helps and sorry about all the UK safety references but I'm
sure there will be similar US regulations.

Good luck

Malcolm

Malcolm Haswell
e.m. unit
Chemispec
School of Health, Natural and Social Sciences
Fleming Building
University of Sunderland
Tyne & Wear
SR1 3SD
UK
e-mail: malcolm.haswell-at-sunderland.ac.uk

----- Original Message -----
X-from: davefissell-at-yahoo.com

Hi,

The short answer is that it takes only 5 PSI of pressure for every 10 feet
(one story tall) of vertical head or drop. So you only need 5 PSI extra to
push "up hill". I am sure you have that much pressure. Suppose the
chiller output is 50 PSI. The pressure at the top of the pipe would be the
output of the chiller under normal SEM conditions minus 5 PSI. You will
gain that 5 PSI back on the drop side of the inverted U tube. So the
pressure at the SEM input should still be 50 PSI. If it's lower than 50,
you could still have an air lock (see below). If you keep your bypass
open, then the pressure will drop. Keep it closed and the SEM on-line
during pressure measurements.
The pressure losses from the delivery lines should be minor unless you use
really small diameter pipes or have a lot of bends. Stick with 1/2" ID
plastic, not copper. Use pipe rated for at least 100 PSI.

Your problem might be in eliminating the initial inverted U loop's air lock
at the top of the loop. You might consider installing a tee and globe
valve at the top of the loop to bleed off *most* of the tapped air.

Paul

At 08:28 AM 1/28/08 -0600, you wrote:
}
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From: nyilmaz-at-mersin.edu.tr
Date: Mon, 28 Jan 2008 13:12:22 -0600
Subject: [Microscopy] Rat corpus callosum formation

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi, we have recently started to work on corpus callosum formation in the
developing mamalian forebrain. First we performed a pilot study to see the
callosol axon projections on E 14 and E 17 mouse foetus brain regarding
the reference studies. We could see the callosal axons on the coronal
sections as shown in the references . But we decided to run the study with
rat foetuses instead of mice because of the lack of the facilities. However
we could not find any spesific timing information in the literature about
CC formation in rats . We wonder when CC spesificly begins and ends to form
during the rat gestation and also where we suppose to see the growing
callosal axons on E 14, 15 and 17 on the coronal histological sections in
rats.



I would greatly appreciate if you could inform me about these issues .



Thank you in advance for any information you can suggest me.



Yours Sincerely

Dr. Necat Yilmaz
Mersin Universitesi Tip Fakultesi
Histoloji ve Embriyoloji Anabilim Dali


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From: garyeaston-at-scannerscorp.com
Date: Mon, 28 Jan 2008 15:34:33 -0600
Subject: [Microscopy] Question about ImageTool

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Anyone know of a plugin for the free image analysis program ImageTool
that will allow it perform automatic particle size and aspect
ratio(height to diameter) calculations? I understand this program can
use Photoshop plugins also. Thanks in advance.


Gary M. Easton


Scanners Corporation
Independent SEM Service
30 years experience
Cambridge SEM's our specialty
410-857-7633



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From: tivol-at-caltech.edu
Date: Mon, 28 Jan 2008 15:35:53 -0600
Subject: [Microscopy] Re: Chiller pump and lifting power.

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html


On Jan 28, 2008, at 6:27 AM, kraftpiano-at-gmail.com wrote:

} I finally got sick of the noise and heat being thrown off by my water
} chiller system for the SEM, so I decided to move it to another room.
} Before I do this, though, the water lines have to be run up into the
} ceiling, over about 20 feet, then down to the microscope again. I've
} taken into consideration the connection end and plumbed in a valve
} system so I have a cut-off to run water through the chiller and piping
} without circulating it through the SEM, but I'm still wondering about
} the lifting power of the pump. Does the power required to lift the
} water lower the flow rate, or does the drop on the other end create
} enough of a siphon effect to cancel out any effects of the lift?
}
} I seem to be able to reason this one out either way, depending on
} which outcome I'm looking for...


Dear Justin,
The chillers for the high-voltage scope in Albany were located in a
sub-sub basement about 10 meters below the lowest point of the scope,
and the water distribution manifold for the lenses was located
another 5 meters above that. There was no difficulty supplying water
to any part of the scope. The pump on the chiller pushed water up to
the manifold, so the height is not a problem, and, as long as there
is no way air can get into the lines, each liter of water pushed into
the line forces one liter to be pushed into the tank, so the water
should circulate the same way regardless of the height it is raised
to. The flow rate can be affected by the length of the lines due to
viscosity; i.e., the pump must provide enough power to overcome the
resistance due to the friction of the water flowing through the
lines, which is higher for longer and thinner lines.
Yours,
Bill Tivol, PhD
EM Scientist
Electron Cryo-Microscopy Facility
Broad Center, Mail Code 114-96
California Institute of Technology
Pasadena CA 91125
(626) 395-8833
tivol-at-caltech.edu


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From: bozzola-at-siu.edu
Date: Mon, 28 Jan 2008 16:05:35 -0600
Subject: [Microscopy] large capacity tap water filters

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

We have been having major problems with our in-line tap water filters
becoming clogged (sometimes on a bi-weekly basis). These
string-filters remove sediment from the tap water that is used to
remove heat from our closed-loop water chillers. Our Physical Plant
has not been able to locate the source of the sludge and we end up
paying them several hundred dollars to come and change two sets of
filters.

Does anyone know of a large capacity (self-cleaning) filtration
system that could be used on the water coming into our small,
microscopy building? Since our major use of water is probably the
water chillers, it may be more advantageous to go this route rather
than relying on the small, under-sink string filters.

Thank you,

John Bozzola
--
+++++++++++++++++++++++++++++++++++++++++++++++++++++++

John J. Bozzola, Ph.D., Director
Integrated Microscopy & Graphics Expertise (IMAGE)
Southern Illinois University
750 Communications Drive - MC 4402
Carbondale, IL 62901
Telephone: 618-453-3730

+++++++++++++++++++++++++++++++++++++++++++++++++++++++

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From: august04-at-verizon.net
Date: Mon, 28 Jan 2008 18:46:05 -0600
Subject: [Microscopy] AskAMicroscopist: Brownian motion

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This Question was submitted to Ask-A-Microscopist by (august04-at-verizon.net)
from http://www.msa.microscopy.org/Ask-A-Microscopist/Ask-A-Microscopist.html on Monday, January 28, 2008 at 18:36:19
Remember to consider the Grade/Age of the student when considering the Question
---------------------------------------------------------------------------
Please reply to both august04-at-verizon.net as well as to the Microscopy Listserver
---------------------------------------------------------------------------

Email: august04-at-verizon.net
Name: Charles Pique

Organization: None

Education: Graduate College

Location: Charleston, West Virginia, USA

Title: Brownian motion

Question: What magnification and conditions are needed to see the brownian motion?


---------------------------------------------------------------------------

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From: gary-at-gaugler.com
Date: Mon, 28 Jan 2008 19:30:09 -0600
Subject: [Microscopy] Re: AskAMicroscopist: Brownian motion

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

As I recall, Brownian motion is in part due to the density
and temperature of particles. The differentiation of
particles is important from large objects (Gouy, 1889).
The smaller the particles, the more impact external
forces have on them. This includes thermal effects.

I think that the basic theory is formulated on particles in a fluid.
If one takes this literally, one could collect rotifers
and examine them under a microscope at perhaps 100X
or less and study their movement. Then, increase the
temperature of their medium and the movement will increase.
The point is that there is no distinct and definitive direction
for movement in either of the thermal conditions. Movement
is random. There is no distinct vector for movement regardless
of temperature.

In particular, the length of the movement is infinite over any length
of interval.
Being rather impossible, Brownian motion is purely an abstract
concept. This is
based on the inability of a particle to move an infinite distance in
a finite length of time. Einstein had some publications about Brownian motion.
You might do some research on/for these.

As an aside, some have identified the movement of employees in a
company as Brownian motion...moving here and there to show activity
but with no actual production output. But that is a stretch (?).

Let us know what you find out.

gary g


At 04:47 PM 1/28/2008, you wrote:
} ----------------------------------------------------------------------------
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of America


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From: john.mardinly-at-intel.com
Date: Mon, 28 Jan 2008 19:52:23 -0600
Subject: [Microscopy] large capacity tap water filters

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

My swimming pool has some very large filters and I can clean them myself
in a half hour. It would require shutting off the microscope, though.
Better to locate the source of sludge.

John Mardinly,

-----Original Message-----
X-from: bozzola-at-siu.edu [mailto:bozzola-at-siu.edu]
Sent: Monday, January 28, 2008 2:06 PM
To: Mardinly, John

We have been having major problems with our in-line tap water filters
becoming clogged (sometimes on a bi-weekly basis). These
string-filters remove sediment from the tap water that is used to
remove heat from our closed-loop water chillers. Our Physical Plant
has not been able to locate the source of the sludge and we end up
paying them several hundred dollars to come and change two sets of
filters.

Does anyone know of a large capacity (self-cleaning) filtration
system that could be used on the water coming into our small,
microscopy building? Since our major use of water is probably the
water chillers, it may be more advantageous to go this route rather
than relying on the small, under-sink string filters.

Thank you,

John Bozzola
--
+++++++++++++++++++++++++++++++++++++++++++++++++++++++

John J. Bozzola, Ph.D., Director
Integrated Microscopy & Graphics Expertise (IMAGE)
Southern Illinois University
750 Communications Drive - MC 4402
Carbondale, IL 62901
Telephone: 618-453-3730

+++++++++++++++++++++++++++++++++++++++++++++++++++++++

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From: john.mardinly-at-intel.com
Date: Mon, 28 Jan 2008 19:55:18 -0600
Subject: [Microscopy] Chiller pump and lifting power.

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Anybody ever heard of a siphon?

John Mardinly


-----Original Message-----
X-from: kraftpiano-at-gmail.com [mailto:kraftpiano-at-gmail.com]
Sent: Monday, January 28, 2008 6:28 AM
To: Mardinly, John

I finally got sick of the noise and heat being thrown off by my water
chiller system for the SEM, so I decided to move it to another room.
Before I do this, though, the water lines have to be run up into the
ceiling, over about 20 feet, then down to the microscope again. I've
taken into consideration the connection end and plumbed in a valve
system so I have a cut-off to run water through the chiller and piping
without circulating it through the SEM, but I'm still wondering about
the lifting power of the pump. Does the power required to lift the
water lower the flow rate, or does the drop on the other end create
enough of a siphon effect to cancel out any effects of the lift?

I seem to be able to reason this one out either way, depending on
which outcome I'm looking for...

--Justin A. Kraft

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From: dac-at-research.umass.edu
Date: Mon, 28 Jan 2008 20:03:23 -0600
Subject: [Microscopy] Re: large capacity tap water filters

Contents Retrieved from Microscopy Listserver Archives
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Hi John,

Our water line currently has one filter and no bypass; on days when
I've had enough coffee to be especially lucid I can change a filter
without the chillers noticing. However it is directly over a 208 3-phase
outlet so while rushing to do the job fast, water drips and I end up
standing in a pool of water while watching it drip into the outlet - not
great.

I sketched out a plan (as yet unimplemented) for a system with 2
alternate branches so that the flow can be switched to an unused filter
unit while the loop with the used filter is isolated and the filter
replaced. I have planned a drain/flush spigot on the inlet side so I can
flush the line upstream of the filters from time to time, or before a
filter change. The standard filters are really cheap at McMaster-Carr (a
couple of dollars, I think; I get a case at a time, we also have
'enriched' water). I can send the Prod# - we use a spun plastic (5um I
think) instead of the string filters.

It is going to be hard to beat the economy of standard mass-produced
filter units for a low volume application supporting some chillers, etc.
If you have the usual 'before and after' pressure gages you can see the
pressure drop developing across the active filter and change filters
before trouble comes knocking.

Dale Callaham
UMASS, Amherst

bozzola-at-siu.edu wrote:
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} We have been having major problems with our in-line tap water filters
} becoming clogged (sometimes on a bi-weekly basis). These
} string-filters remove sediment from the tap water that is used to
} remove heat from our closed-loop water chillers. Our Physical Plant
} has not been able to locate the source of the sludge and we end up
} paying them several hundred dollars to come and change two sets of
} filters.
}
} Does anyone know of a large capacity (self-cleaning) filtration
} system that could be used on the water coming into our small,
} microscopy building? Since our major use of water is probably the
} water chillers, it may be more advantageous to go this route rather
} than relying on the small, under-sink string filters.
}
} Thank you,
}
} John Bozzola

==============================Original Headers==============================
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From: jtwilley-at-sprynet.com
Date: Mon, 28 Jan 2008 20:03:58 -0600
Subject: [Microscopy] Re: AskAMicroscopist: Brownian motion

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Charles,

In my experience a rock thin section consisting mostly of quartz will
offer opportunities to see this at magnifications of about 400x and above
- occasionally even lower. Quartz that is formed hydrothermally (by
crystalization from silica-bearing water deep in the earth) typically
contains fluid inclusions. These are visible as voids inside the quartz.
Often they are not completely filled by liquid and the remaining space is
occupied by a bubble of gas. Brownian motion will be apparent from the
agitation of the bubble--- it will appear to be constantly jostled about
by some unseen forces. If the heat from the microscope illuminator is not
completely eliminated by a filter, the jostling will become more violent
as the thin section warms up and decrease when the light is removed for a
time.

You will need to view the thin section in transmitted light but it is not
necessary to have an actual petrographic microscope to see the effect, a
biological scope will do. Some other stone sections will exhibit
two-phase (gas-liquid) inclusions. Calcite, for example may contain
gas-liquid inclusions or liquid-liquid inclusions. The latter consist of
immiscible liquids such as brine and petroleum. However, the low mass of
a gas bubble in a fluid inclusion makes it a better candidate to observe
the motion and quartz more often provides a clear view.

John Twilley
Conservation Scientist

On Mon, 28 Jan 2008 19:46:21 -0500, {august04-at-verizon.net} wrote:

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} Email: august04-at-verizon.net
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}
} Organization: None
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} Education: Graduate College
}
} Location: Charleston, West Virginia, USA
}
} Title: Brownian motion
}
} Question: What magnification and conditions are needed to see the
} brownian motion?
}
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From: beaurega-at-westol.com
Date: Mon, 28 Jan 2008 21:09:41 -0600
Subject: [Microscopy] Re: large capacity tap water filters

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

John,

I agree with Dale. You should change your own filters, if possible. I
have seen the dual in-line filter and switching setups used in plants that
he described. Get filters with a pressure relief button to make changing
cartridges easier.

The real questions are, "What is plugging the (cartridge?) filter and what
is the size of the 'dirt'? Once you know the ID, from TEM for example,
then you might be able to find the source or cause.

McMaster-Carr shows a fiberglass unit very similar to a water softener. It
is a 'sediment and dirt' filter unit with a back wash timer. It is item
9843K11, ~$400. It says, "Rated at 50 microns."

You could try to rent one from a water softener company with the option to
buy. If you are lucky, a large dealer will have softener units used in
apartments for a short periods of time that are quite new and half the
price. I did that to get a year old iron filter that used KMnO4. I also
bought a used water softener that had the resin and sand changed out by the
dealer. Both worked just fine.

Paul

At 04:06 PM 1/28/08 -0600, you wrote:
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From: kenner.rita-at-marshfieldclinic.org
Date: Mon, 28 Jan 2008 22:40:34 -0600
Subject: [Microscopy] viaWWW: Zeiss EM 900

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Email: kenner.rita-at-marshfieldclinic.org
Name: Rita Kenner

Organization: Marshfield Clinic, Marshfield WI. 715-387-9159

Title-Subject: [Filtered] Zeiss EM 900

Question: Does anyone happen to know the going price/value of a 14 year old Zeiss EM900 electron microscope? (My facility is planning to purchase a CCD camera for this particular scope, but then 2 or 3 years down the road, is planning on purchasing an entirely new scope altogether. In my humble opinion, it would make more sense to buy the new scope now, complete with the digital camera, so as not to try to retro-fit a camera we buy now for the Zeiss, onto a scope that may not be a Zeiss.)
Thanks in advance for your time and perspectives.
Rita Kenner

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From: Elliott-at-arizona.edu
Date: Tue, 29 Jan 2008 06:32:29 -0600
Subject: [Microscopy] imuno-gold TEM analysis

Contents Retrieved from Microscopy Listserver Archives
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Hi Listers
I am doing an analysis of some immuno-TEM. I am interested in the
enrichment of gold particles on a membrane. I am probing a
transmembrane protein with an IgG and then a secondary (gold labeled)
IgG.
What I am thinking is to count the gold particles that are within X nm
of the membranes in question and the gold that is not within X
distance of the membrane. Then define enrichment as;


(# gold within X nm of membrane)/(length of membrane * (2 * X))
__________________________________________________

(# gold particles in field)/(area of field)

My questions are;
1) does this make sense?
2) am I reinventing the wheel (I assume yes :-)
3) if 'yes' to #2, where should I go for info
4) (most important of all) what is the value of X?

Thank you
David

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From: nizets2-at-yahoo.com
Date: Tue, 29 Jan 2008 07:48:51 -0600
Subject: [Microscopy] AskAMicroscopist: Brownian motion

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi!

Any "scientific" light microscope will suffice. Just look at a suspension of bacteria at 40x or 100x objective (at 40x the bacteria are just very tiny spots but you can see them moving) and you will see them dancing around. If flagella are involved in the movement, they have a faster and more regular movement like turning in circles or rushing fast through the field of view. By extension, any particle with a size close to bacteria can be visualized as well, like the debris usually present in eucaryotic cell cultures, fine dusts...

Best regards,

Stephane


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Sent: Tuesday, January 29, 2008 1:51:29 AM

This Question was submitted to Ask-A-Microscopist by (august04-at-verizon.net)
from http://www.msa.microscopy.org/Ask-A-Microscopist/Ask-A-Microscopist.html on Monday, January 28, 2008 at 18:36:19
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Name: Charles Pique

Organization: None

Education: Graduate College

Location: Charleston, West Virginia, USA

Title: Brownian motion

Question: What magnification and conditions are needed to see the brownian motion?


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From: tjzhang-at-umd.edu
Date: Tue, 29 Jan 2008 08:45:41 -0600
Subject: [Microscopy] viaWWW: Help please: ESEM-E3

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Email: tjzhang-at-umd.edu
Name: Tim

Organization: UMD

Title-Subject: [Filtered] Help please: ESEM-E3

Question: Dear All,

There is an ESEM E3 in our lab that is over 15 years old but runs well.

Last week, I found the battery on CPU board runs out. I have ordered the battery on line but I need to re-load the "start software". I wonder who has this kind of software and how to send it to RAM memory on CUP board?

Thank you very much in advance.

Tim


Login Host: 128.8.139.35
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From: eschumacher-at-mccrone.com
Date: Tue, 29 Jan 2008 08:46:00 -0600
Subject: [Microscopy] After-Market Service for Ultracut Microtomes

Contents Retrieved from Microscopy Listserver Archives
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Greetings Fellow Microscopists,

There were some recent postings regarding service and maintenance of
older Ultracut and Ultracut E microtomes. I didn't see any responses
providing resources for after-market service in the Midwest area, and so
I'm raising the question again. Is there anyone reasonably near the
Chicago area who provides service for both ambient and cryo units?

Thanks in advance,

Elaine


Elaine Schumacher
Senior Research Scientist
McCrone Associates, Inc.
850 Pasquinelli Drive
Westmont,IL 60559-5539 USA
630-887-7100 (tel)
630-887-7417 (fax)
E-mail: eschumacher-at-mccrone.com
Web Site: www.mccrone.com




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From: beth-at-plantbio.uga.edu
Date: Tue, 29 Jan 2008 09:25:25 -0600
Subject: [Microscopy] Re: After-Market Service for Ultracut Microtomes

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi Elaine,
I use David Benjamin {dbenjamin-at-dbmicroservice.com} . He is based in
the Atlanta area so this info may not seem helpful but Airtran has
many direct flights to your area. He's a good serviceman for
microtomes, cryostats, and microscopes.

best,
Beth

On Jan 29, 2008, at 9:46 AM, eschumacher-at-mccrone.com wrote:

}
}
}
} ----------------------------------------------------------------------------
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of
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} On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} ----------------------------------------------------------------------------
}
} Greetings Fellow Microscopists,
}
} There were some recent postings regarding service and maintenance of
} older Ultracut and Ultracut E microtomes. I didn't see any responses
} providing resources for after-market service in the Midwest area,
} and so
} I'm raising the question again. Is there anyone reasonably near the
} Chicago area who provides service for both ambient and cryo units?
}
} Thanks in advance,
}
} Elaine
}
}
} Elaine Schumacher
} Senior Research Scientist
} McCrone Associates, Inc.
} 850 Pasquinelli Drive
} Westmont,IL 60559-5539 USA
} 630-887-7100 (tel)
} 630-887-7417 (fax)
} E-mail: eschumacher-at-mccrone.com
} Web Site: www.mccrone.com
}
}
}
}
} ==============================Original
} Headers==============================
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From: tbargar-at-unmc.edu
Date: Tue, 29 Jan 2008 09:29:00 -0600
Subject: [Microscopy] Can hardened fixed tissue be "softened" by Microwave treatment?

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html


I've got a surgeon who is working with human livers that are very hard from
the embalming process and he had heard that microwaving tissue may soften
up the tissue and make it easier to cut. I'm going to let him use my
Biowave and try different wattages. I have never heard of this effect
before. Has anybody out there heard of or actually know if hardened fixed
tissue can be softened by microwaves. Thanks, all help is appreciated.

Tom Bargar
University of Nebraska Medical Center
Core Electron Microscopy Research Facility
986395 Nebraska Medical Center
Omaha, NE 68198-6395
402-559-7347
tbargar-at-unmc.edu


==============================Original Headers==============================
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From: bozzola-at-siu.edu
Date: Tue, 29 Jan 2008 14:05:00 -0600
Subject: [Microscopy] Re: AskAMicroscopist: Brownian motion

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Brownian motion is readily demonstrated using small particles in an
aqueous phase. For example, India ink (consisting of carbon black
particles) can be observed under high magnification (500X and above)
to see the random movement of the black particles. The particles seem
to "shiver" or "quake" and sometimes move off in random directions.
If you have phase contrast (or darkfield), this would enhance the
viewing. If not, then try offsetting the substage condenser so that
the light is coming in at an angle.

--
+++++++++++++++++++++++++++++++++++++++++++++++++++++++

John J. Bozzola, Ph.D., Director
Integrated Microscopy & Graphics Expertise (IMAGE)
Southern Illinois University
750 Communications Drive - MC 4402
Carbondale, IL 62901
Telephone: 618-453-3730

+++++++++++++++++++++++++++++++++++++++++++++++++++++++

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From: probe-at-geotrack.com.au
Date: Wed, 30 Jan 2008 00:47:29 -0600
Subject: [Microscopy] zeiss axioplan microscope

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

I am interested in buying a zeiss axioplan microscope, (late 80's early
90's) or later model axiotron if available. If anyone has one they would
like to sell or know of a source I would greatly appreciate a reply. Off
line is probably best.
Cheers
Pat


Patrick R Kelly Operations Manager
Geotrack International Pty Ltd ABN16 006 821 209
37 Melville Road, Brunswick West, Victoria 3055 Australia
Telephone: +613 93801077 Facsimile: +613 93801477
email: mail-at-geotrack.com.au
web: http://www.geotrack.com.au


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From: vhacopian-at-wellesley.edu
Date: Wed, 30 Jan 2008 07:36:09 -0600
Subject: [Microscopy] TEM - negative scanners

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

I wish to purchase a flatbed scanner for TEM negatives. I have received
recommendations for the Canon 9950F and the Epson V750-M. The former may
no longer be available, as it is not listed on the Canon web site--only
the 8800F is. Any suggestions would be welcome and highly appreciated.
Vachik Hacopian


==============================Original Headers==============================
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From: nizets2-at-yahoo.com
Date: Wed, 30 Jan 2008 09:00:54 -0600
Subject: [Microscopy]

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Dear listers,

We just changed the IGP pump of the gun chamber only 4 years after the installation of our Tecnai G20. This change was advised by a FEI engineer.
We do not even have 400 working hours on this machine and I wondered if it was normal that we already have to change the pump.
We work mainly with ultrathin sections of biological probes embedded in Epon. They are pretty contaminated with carbon, as evidenced by light circles remaining on the sections after even a very short illumination time (I am usually working at 120 kV, LaB6). I am wondering if this carbon contamination, evaporated by the electron beam, is not at least partly responsible for the dirtiness of the pumps (the pump of the column is bigger than the one for the gun, which would explain why it was not so dirty). If this is the case, perhaps a plasma cleaner would not only be a convenience for me but could bring a financial advantage for my boss (I know you see what I mean ;-)).
What would be the cost of a plasma cleaner?
What is your opinion on the question? Do you think that a plasma cleaner would increase the lifetime of the IGPs?

Best regards,

Stephane


____________________________________________________________________________________
Looking for last minute shopping deals?
Find them fast with Yahoo! Search. http://tools.search.yahoo.com/newsearch/category.php?category=shopping

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From: marksmsa-at-gmail.com
Date: Wed, 30 Jan 2008 12:46:52 -0600
Subject: [Microscopy] Postdoctoral Position

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Postdoctoral position at Northwestern University
DFT and Electron Microscopy

A postdoctoral position is available at Northwestern University
for someone with expertise in both DFT (Wien2k, Vasp, PWSCF) and
transmission electron microscopy. The research will be in a number
of different areas including charge density measurements at both
surfaces and for bulk materials; structure and energies of surface
reconstructions; oxides for use either as catalysts or in solid
oxide fuel cells. The applicant must hold a recent Ph.D. in physics,
chemistry, or materials science. Further requirements for this position
are: (1) A good knowledge of electronic structure theory. (2) Experience
with first-principles calculations such as Density Functional Theory. (3)
Extensive hands-on experience with transmission electron microscopy and
diffraction (4) Ability to communicate effectively with coworkers and
collaborators. (5) Demonstrated ability to write high-quality manuscripts
suitable for publication in peer-reviewed journals.


--
Laurence Marks
Department of Materials Science and Engineering
MSE Rm 2036 Cook Hall
2220 N Campus Drive
Northwestern University
Evanston, IL 60208, USA
Tel: (847) 491-3996 Fax: (847) 491-7820
email: L-marks at northwestern dot edu
Web: www.numis.northwestern.edu
EMM2007 http://ns.crys.ras.ru/EMMM07/
Commission on Electron Diffraction of IUCR
www.numis.northwestern.edu/IUCR_CED

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From: marksmsa-at-gmail.com
Date: Wed, 30 Jan 2008 12:56:47 -0600
Subject: [Microscopy] Postdoctoral Position in Nanoscale Tribology

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Postdoctoral position at Northwestern University
In-Situ Tribology at the Nanoscale

A postdoctoral position is available at Northwestern University
for someone with expertise in mechanical properties at the nanoscale and
transmission electron microscopy, and the ability to do materials modelling.
The research will involve extending established dislocation and deformation
models used for grain boundaries and interfaces in strong materials to weak
interfaces relevant to tribological applications [1-3]. For instance, the work
might involve testing the limits of applying conventional models for restricting
the motion of dislocations due to point defects in the bulk to the problem of
point defects at the interface of two sliding materials. The applicant
must hold a
recent Ph.D. in physics, chemistry, or materials science with a preference for
materials science. Further requirements for this position are: (1) A
good knowledge
basic mechanical properties at the atomistic nanoscale. (2) Some experience
with transmission electron microscopy and diffraction in order to
collaborate with
others doing more experimental work 3) Ability to communicate effectively with
coworkers and collaborators. (5) Demonstrated ability to write
high-quality manuscripts
suitable for publication in peer-reviewed journals.

Interested applicants should contact L-marks -at- northwestern.edu and send a CV
including the names of referees as well as a 1 page outline of how
they might use
core materials science mechanical property formalism's and theories to
model tribological
processes at the nanoscale?

1. A. P. Merkle and L. D. Marks, Tribology Letters 26 73 (2007)
2. A. P. Merkle and L. D. Marks, Philosophical Magazine Letters, 87, 527 (2007)
3. A. P. Merkal and L. D. Marks, Appl Phys Letts 90, 064101 (2007)

--
Laurence Marks
Department of Materials Science and Engineering
MSE Rm 2036 Cook Hall
2220 N Campus Drive
Northwestern University
Evanston, IL 60208, USA
Tel: (847) 491-3996 Fax: (847) 491-7820
email: L-marks at northwestern dot edu
Web: www.numis.northwestern.edu
EMM2007 http://ns.crys.ras.ru/EMMM07/
Commission on Electron Diffraction of IUCR
www.numis.northwestern.edu/IUCR_CED

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From: eschumacher-at-mccrone.com
Date: Wed, 30 Jan 2008 13:05:12 -0600
Subject: [Microscopy] Summary of Suggestions for Microtome Service

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Greetings Fellow Microscopists,

Here are the leads that were suggested for possible servicing of older
Ultracut microtomes. You may find some of them to be useful for other
types of equipment service as well.

Tek-Net, Jon Petz, Lakewood, NJ, 732-905-5530
They send a crate for shipment of the equipment, which you return to
them when you get the repaired unit back.

David Benjamin, dbenjamin-at-dbmicroservice.com, Atlanta, GA

Sercomp International, www.sercompintl.com

Please note that I haven't investigated any of these resources yet for
my specific Ultracut issues, but I wanted to share the information.
Thanks very much to all who replied to my posting.

Regards,

Elaine


Elaine Schumacher
Senior Research Scientist
McCrone Associates, Inc.
850 Pasquinelli Drive
Westmont,IL 60559-5539 USA
630-887-7100 (tel)
630-887-7417 (fax)
E-mail: eschumacher-at-mccrone.com
Web Site: www.mccrone.com


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From: tivol-at-caltech.edu
Date: Wed, 30 Jan 2008 14:17:14 -0600
Subject: [Microscopy] Re:

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html


On Jan 30, 2008, at 7:01 AM, nizets2-at-yahoo.com wrote:

} We just changed the IGP pump of the gun chamber only 4 years after
} the installation of our Tecnai G20. This change was advised by a
} FEI engineer.
} We do not even have 400 working hours on this machine and I
} wondered if it was normal that we already have to change the pump.
} We work mainly with ultrathin sections of biological probes
} embedded in Epon. They are pretty contaminated with carbon, as
} evidenced by light circles remaining on the sections after even a
} very short illumination time (I am usually working at 120 kV,
} LaB6). I am wondering if this carbon contamination, evaporated by
} the electron beam, is not at least partly responsible for the
} dirtiness of the pumps (the pump of the column is bigger than the
} one for the gun, which would explain why it was not so dirty). If
} this is the case, perhaps a plasma cleaner would not only be a
} convenience for me but could bring a financial advantage for my
} boss (I know you see what I mean ;-)).
} What would be the cost of a plasma cleaner?
} What is your opinion on the question? Do you think that a plasma
} cleaner would increase the lifetime of the IGPs?


Dear Stephane,
The IGP is on full time, so even though there have been few hours
that the instrument was in use, the pump has been working for the
entire 4 years. This is still a short period, especially since there
are relatively few contaminants in the gun volume (or should be).
The mechanism of ion pumps is that residual gas is ionized and the
ions are accelerated by an electric field and become embedded in the
getter, which can get filled to the extent that any additional ion
incident on the getter will dislodge an ion that is already there.
The lifetime, therefore, depends on how good the vacuum is and how
large the surface of the getter is. Other things that can shorten
pump lifetime are the presence of water in the column--which is not
likely to be an issue for your usage and is more of a problem in
cryoEM--and the formation of spurs on the getter surface. The
indication for pump replacement is loss of performance, so if your
vacuum is poor, where it had been good, then the pump should be
replaced (assuming that a vacuum leak has not developed). I doubt
that carbon is the problem, but I could be wrong about that. A
plasma cleaner can remove contamination from the column, which will
give you a cleaner instrument and a better vacuum, which, in turn,
will increase pump lifetime, but I don't know whether that will be
enough to cover the cost--I'll let the manufacturers of these systems
answer that question.
Yours,
Bill Tivol, PhD
EM Scientist
Electron Cryo-Microscopy Facility
Broad Center, Mail Code 114-96
California Institute of Technology
Pasadena CA 91125
(626) 395-8833
tivol-at-caltech.edu


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From: bozzola-at-siu.edu
Date: Wed, 30 Jan 2008 14:50:02 -0600
Subject: [Microscopy] Re: ion pump longevity

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

I've been following this discussion with interest since I have never
had an instrument with IGP's. I'm surprised to find that IGP's have a
(sometimes rather) limited lifetime. When you say they need to be
replaced, do you mean just the adsorptive surfaces or the entire
sealed system? How much does this cost? A ballpark figure is fine. I
need this information for planning and teaching purposes.

Thank you,

John Bozzola
Integrated Microscopy & Graphics Expertise (IMAGE)
Southern Illinois University
750 Communications Drive - MC 4402
Carbondale, IL 62901
Telephone: 618-453-3730


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From: gary-at-gaugler.com
Date: Wed, 30 Jan 2008 15:24:51 -0600
Subject: [Microscopy] Re: Re: ion pump longevity

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Not seeing a discussion of bakeout, I'd bring that up.

New generation pumps have built-in bakeout coils and
instrument vacuum connections also have a bakeout coil
surrounding each one. These pumps are essential for
high vacuum that is highly beneficial for LaB6 cathodes
and especially critical for FE systems. For W systems,
I have never seen an IGP unless it was set up to handle
both W and LaB6.

Depending on the use of the system, eventually the gun
chamber will become contaminated with gas and always
does when the cathode or FE tip is changed. Part of the
changeout process is to bakeout the gun chamber, IGPs
and vacuum connections (the connections with a gazillion
bolts like between IGP and column/chamber). During this
time, isolation valves that seal off the column and the
gun chamber are opened while baking so the main vacuum
system pulls the junk out. When done, the valves are
closed and IGPs start pulling the vacuum down further.

During the bakeout process, the junk in the Ta and Ti
parts of the IGP also get dislodged and dumped. This
can be a separate part of "recycling" an IGP that is
staturated but not requiring repair. When the IGP
needs repair/rebuild, the whole thing (minus magnet)
is sent off for rebuild or exchange. The following
list from Duniway gives some typical costs for this.

http://www.duniway.com/images/pdf/pg/p-42-var-style-rebuilt.pdf

I have not seen prices or services for the newer IGPs.

Older tools that do not have bakeout coils built-in can
still be baked using off the shelf heating coil tape.
They are rated in watts, width and length and are controlled
by a simple thermal feedback box. These units are typically
around $500 or less and can save lots of bucks if a simple
bakeout is all that is needed from time to time--and with
cathode/filament change.

With bakeout when the gun is changed and with reasonable care,
my experience is that IGPs last for many years...perhaps
up to ten years of continuous service. But of course, there
is always the flakey one that does develop a flake and
trips the IGP power supply and must be replaced.

gary g.



At 12:51 PM 1/30/2008, you wrote:




} ----------------------------------------------------------------------------
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of America


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17, 20 -- From: Gary Gaugler {gary-at-gaugler.com}
17, 20 -- Subject: Re: [Microscopy] Re: ion pump longevity
17, 20 -- Cc: MSA listserver {microscopy-at-microscopy.com}
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From: tivol-at-caltech.edu
Date: Wed, 30 Jan 2008 15:27:08 -0600
Subject: [Microscopy] Re: Re: ion pump longevity

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On Jan 30, 2008, at 12:50 PM, bozzola-at-siu.edu wrote:

} I've been following this discussion with interest since I have never
} had an instrument with IGP's. I'm surprised to find that IGP's have a
} (sometimes rather) limited lifetime. When you say they need to be
} replaced, do you mean just the adsorptive surfaces or the entire
} sealed system? How much does this cost? A ballpark figure is fine. I
} need this information for planning and teaching purposes.


Dear John,
For the ion pumps I've dealt with, the getter assembly is replaced.
This is the plates and whatever holds them at the proper separation.
I've sent the pump back to the EM manufacturer and gotten a
refurbished pump back. I have had only very limited experience with
this, however, because the ion pumps on the HVEM were very large with
correspondingly large capacity and didn't need replacing for the
entire 20+ years I was in Albany, and the pump in our FEG here at
Caltech was covered by the service contract. Apparently it developed
a whisker on the getter, the symptoms of which were that the vacuum
would get bad fairly quickly and shut the FEG off. This happened
every few months until the problem was diagnosed.
Yours,
Bill Tivol, PhD
EM Scientist
Electron Cryo-Microscopy Facility
Broad Center, Mail Code 114-96
California Institute of Technology
Pasadena CA 91125
(626) 395-8833
tivol-at-caltech.edu


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From: larry.ackerman-at-ucsf.edu
Date: Wed, 30 Jan 2008 16:07:41 -0600
Subject: [Microscopy] Re: TEM - negative scanners

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If the negtive is just slightly denser than "normal" the Canon scanner
cannot give a good full tonal scan. The D-Max is insufficient. I have
not tried the Epson
Larry

vhacopian-at-wellesley.edu wrote:
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}
} I wish to purchase a flatbed scanner for TEM negatives. I have received
} recommendations for the Canon 9950F and the Epson V750-M. The former may
} no longer be available, as it is not listed on the Canon web site--only
} the 8800F is. Any suggestions would be welcome and highly appreciated.
} Vachik Hacopian
}
}
} ==============================Original Headers==============================
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}

--
Larry Ackerman, Associate Specialist
UCSF, Dept. of Anatomy, Rm S1347
513 Parnassus Ave., Box 0452
San Francisco, CA 94143

larry.ackerman-at-ucsf.edu


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From: sandra.gardner-at-xerox.com
Date: Wed, 30 Jan 2008 16:41:02 -0600
Subject: [Microscopy] viaWWW: 2 questions concerning microtomy of thin films

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Email: sandra.gardner-at-xerox.com
Name: Sandra Gardner

Organization: Xerox Research Centre of Canada

Title-Subject: [Filtered] 2 questions concerning microtomy of thin films

Question: I have a multi layer film in which one of the layers is water soluble. We want to cross section the sample for TEM to view the various layers, each of which are less than 500nm thick. The total thickness of the plastic substrate plus multilayer film is aprox. 500microns (the substate is aprox 300microns of this). I've embedded the film in a epoxy resin for sectioning. I don't know how to go about capturing thin sections ( {100nm) if I can't put water in the boat. I could cut them dry, but again, I'm not sure how to transfer them to the grid. I am using a Diatome diamond knife. Any suggestions would be greatly appreciated.

Another question I have regards the use of tape as a support media for cryo-sectioning. Many of our samples are films which I typically embed in epoxy resin. We now have cryo-sectioning capabilities and i would like to simply sandwich my film between tape and cryo cut thin films for TEM analyses. Is there any tape which has good adhesion properties at -120C and stand up well for TEM (glue does not interfere with sample)

Again, any direction is appreciated!

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From: hadden-at-wingate.edu
Date: Wed, 30 Jan 2008 16:41:32 -0600
Subject: [Microscopy] viaWWW: vacuum problems JEOL JSM5600LV SEM

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Email: hadden-at-wingate.edu
Name: Lee Hadden

Organization: Wingate University

Title-Subject: [Filtered] vacuum problems JEOL JSM5600LV SEM

Question: Our JEOL 5600lv SEM does not attain operating vacuum. It goes through the PRE-EVAC and into the EVAC modes in normal time frame, but remains in EVAC, never going to READY for specimen observation. Any ideas for fixing the problem? Cooling water temp and flow rate OK as are DP temp and oil. The column will hold a vacuum for weeks + even with the SEM off.

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From: connellyps-at-nhlbi.nih.gov
Date: Wed, 30 Jan 2008 17:07:08 -0600
Subject: [Microscopy] Re: Interest in smaller "Permanox" dishes?-Results

Contents Retrieved from Microscopy Listserver Archives
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It has been a week since my posting. I received 7 replies.

All replies were in favor of smaller dishes with one stating that 96 wells
would be even better for his work.

I do not think that this is a large enough group of potential customers for
the any company to consider it a valid request to make such a product.

The reason that I did not like the chamber slides was that there was so
little flat area when I embedded the cells in a 4 well configuration. I also
forgot to use LX-112 (Ladd) in my Epon formula instead of EM-Bed812
(Electron Microscopy Sciences) so the sides of the wells melted a bit making
it very hard to get the sides off the polymerized Epon blocks. Perhaps I'll
try removing the sides before embedding the next time and use the slide
duplicating mold to hold the Epon onto the Permanox slide for curing or get
some 2 well chambered slides.

One person, Stephane, asked where I got the 60mm dishes. My supplier is
Electron Microscopy Sciences but I believe other suppliers may also carry
them.

Thank you for participating.
Pat

} For quite some time I have wondered why NUNC did not make a Permanox Petri
} Dish smaller than 60 x 15 mm. I have grown to really appreciate the
} advantages of using the Permanox over standard Polystyrene dishes for tissue
} cultured cells grown for TEM experiments since every cell line that I have
} tried adheres well to them, they can withstand chemicals like acetone and
} propylene oxide that dissolve the polystyrene and the embedded cells come
} away from the Permanox so easily and smoothly.
}
} With the special cells and reagents that I am now using for TEM, it is a big
} waste to grow cells over such a large area when a 35 x 15 mm dish would do
} nicely. I do want a dish not a chambered slide.
}
} I would like to know if there are others (you)
} 1. who would switch to a smaller dish if they would be made available.
} (this is my pick)
} 2. who would like to use both the 60mm and 35mm dishes
} 3. who would only use the 60mm dishes
} If I get a reasonable response I will contact the company with my results to
} back up my request that they consider making the smaller dishes.
}
} Comments are welcome.
}
} For the survey, it may be best to answer me "Off-ListServer" so as not to
} fill up the emails of other members. I will let the ListServer know the
} tally after the replies come in.
}
} Patricia Stranen Connelly
} Biologist, Electron Microscopy
} NHLBI Electron Microscopy Core
} National Institutes of Health
} 14 Service Road South
} Bldg. 14E ­ Rm. 111B MSC 5570
} Bethesda, MD 20892-5570
} Phone 301-496-3491
} FAX 301-480-6560
} connellyps-at-mail.nih.gov



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From: cervantes-at-bendres.com
Date: Wed, 30 Jan 2008 19:38:05 -0600
Subject: [Microscopy] viaWWW: 2 questions concerning microtomy of thin

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Sandra -

I also work with water soluble materials, and so often have to cut dry.
I have found that a diamond knife is preferable to glass (less "sticky"
so sections are easier to get off the knife surface), but that may be
something you want to experiment with. To transfer sections from the
knife to the grid, I use an eyelash probe (I buy mine from Ted Pella,
but people make them as well). It takes a little practice, but that is
what works best for me. I also use the probe to gently "flatten" the
sections onto the grid surface (I use 300 mesh Copper grids with Formvar
support film).

Diatome used to make a Cryo P diamond knife (don't know if they still
do) with a special platform that makes it easier to transfer sections.
This has been my favorite knife for dry-sectioning.

Sorry can't help with your second question, but hope this was useful.

Jessica

____________________
Jessica Cervantes
Bend Research Inc
64550 Research Rd
Bend, OR 97701
www.bendres.com





-----Original Message-----
X-from: sandra.gardner-at-xerox.com [mailto:sandra.gardner-at-xerox.com]
Sent: Wednesday, January 30, 2008 2:49 PM
To: Cervantes, Jessica

This Question/Comment was submitted to the Microscopy Listserver
using the WWW based Form at
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Email: sandra.gardner-at-xerox.com
Name: Sandra Gardner

Organization: Xerox Research Centre of Canada

Title-Subject: [Filtered] 2 questions concerning microtomy of thin films

Question: I have a multi layer film in which one of the layers is water
soluble. We want to cross section the sample for TEM to view the
various layers, each of which are less than 500nm thick. The total
thickness of the plastic substrate plus multilayer film is aprox.
500microns (the substate is aprox 300microns of this). I've embedded
the film in a epoxy resin for sectioning. I don't know how to go about
capturing thin sections ( {100nm) if I can't put water in the boat. I
could cut them dry, but again, I'm not sure how to transfer them to the
grid. I am using a Diatome diamond knife. Any suggestions would be
greatly appreciated.

Another question I have regards the use of tape as a support media for
cryo-sectioning. Many of our samples are films which I typically embed
in epoxy resin. We now have cryo-sectioning capabilities and i would
like to simply sandwich my film between tape and cryo cut thin films for
TEM analyses. Is there any tape which has good adhesion properties at
-120C and stand up well for TEM (glue does not interfere with sample)

Again, any direction is appreciated!

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From: fvillalovoz-at-deltacollege.edu
Date: Wed, 30 Jan 2008 20:16:36 -0600
Subject: [Microscopy] viaWWW: Job opening, E.M. Faculty

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Email: fvillalovoz-at-deltacollege.edu
Name: Frank Villalovoz

Organization: San Joaquin Delta College

Title-Subject: [Filtered] Job opening, E.M. Faculty

Question: San Joaquin Delta College is currently seeking candidates for a full-time faculty position in electron microscopy with experience in the biological sciences. The successful candidate should have a strong background in sample preparation for both the TEM and SEM. The position requires individual training of students in microscope operation, ultramicrotomy, critical point drying and all related biological techniques. Teaching responsibilities also
include light and electron optics, digital imaging, and other aspects of microscopy as needed. Degree requirements and salary are dependent upon experience.

San Joaquin Delta College in Stockton, California has a two-year training program that has been training students for almost 40 years. It is one of only two programs in the nation at the community college level. We currently have four SEMs, three TEMs, one FIB, a new AFM, and a compliment of biological and materials sample preparation instrumentation. The facility has 18,000 square feet.

Applications and a job description can be obtained at
http://www.deltacollege.edu

Application information can be obtained from
Jackie Layman, Human Resources, email: jlayman-at-deltacollege.edu (209) 954-5058

For additional information about the laboratory contact:

Frank Villalovoz, faculty, email: fvillalovoz-at-deltacollege.edu (209) 954-5249
Cathy Davis, Lab supervisor, email: cdavis-at-deltacollege.edu (209) 954-5246

Center for Microscopy and Allied Sciences
San Joaquin Delta College
5151 Pacific Avenue
Stockton, California, 95207


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From: ramshes-at-musc.edu
Date: Wed, 30 Jan 2008 20:39:31 -0600
Subject: [Microscopy] viaWWW: Second Charleston Workshop on LIGHT MICROSCOPY FOR THE

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Email: ramshes-at-musc.edu
Name: Venkat Ramshesh

Organization: Medical University of South Carolina

Title-Subject: [Filtered] Announcement: LIGHT MICROSCOPY FOR THE BIOSCIENCES (LMB)

Question: Second Charleston Workshop on

LIGHT MICROSCOPY FOR THE BIOSCIENCES (LMB)

Medical University of South Carolina

May 18-23, 2008

The Second Charleston Workshop on LIGHT MICROSCOPY FOR THE BIOSCIENCES (LMB) Workshop provides a solid introduction to the concepts and practical applications of light microscopy relevant to modern cell and molecular biology. Students will have opportunities for extensive hands-on experience with state-of-the-art equipment for optical imaging,digital image processing, and fluorescence and confocal/multiphoton
microscopy guided by experienced academic and commercial faculty. Lectures and laboratory exercises will include: optics of image formation; microscope alignment; phase contrast and differential interference contrast microscopy; video and digital cameras; contrast enhancement by analog and digital image processing; principles of fluorescence and fluorescence microscopy; ion imaging and fluorescent probes, including green fluorescent protein; fluorescence resonance
energy transfer; and laser scanning confocal and multiphoton microscopy. A commercial faculty representing leading microscope manufacturers will make available for student use the latest and most advanced instrumentation for light microscopy, image detection and computerized image analysis. The LMB Workshop is designed for doctoral level scientists, advanced pre-doctoral students and high level technical
personnel. No prior experience with microscopy is required. All students will benefit from in-depth interaction with instructors. Students are encouraged to bring their own specimens for analysis.


Tuition: $750.00

Application Deadline: April 1, 2008

Principal Instructors:

John J. Lemasters, M.D., Ph.D., Organizer

P. Darwin Bell, Ph.D.

Prakash Kara, Ph.D.

Margaret Kelly, Ph.D.

Peter Komlosi, Ph.D.

Anna-Liisa Nieminen, Ph.D.

Venkat Ramshesh, Ph.D.


To apply, send a curriculum vita and a brief letter describing your research interests and reasons for enrolling. Because the course is expected to be oversubscribed, applicants should inquire as soon as
possible. Please indicate your complete mailing address, telephone/fax number and email address. Full consideration will be given to applications received by April 1, 2008.


For further information or to apply, contact:

Venkat K Ramshesh
Medical University of South Carolina
Center for Cell Death, Injury and Regeneration and Hollings Cancer
Center
280 Calhoun Street, PO Box 250140
Charleston, SC 29425
Telephone (843) 792- 3530, FAX (843) 792-1617
E-mail: ramshes-at-musc.edu

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From: jacques.faerber-at-ipcms.u-strasbg.fr
Date: Thu, 31 Jan 2008 03:18:52 -0600
Subject: [Microscopy] Re: ion pump longevity

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Hi all

A few cents too : as other have point out, the two main points are :

-at what vacuum levels has the pump worked ? If it works allways at
-7 mbar or less, it will be earlier tired, by sputtering it Ti, building
a conductive film on it insultors (leakage current, that means than even
with a very good vacumm, one has a ion current from microamps to tenth
of microamps), memory effects (giving pressure bursts which may shut off
the gun, mmmmmmh !), and slow pumping rate. If it has worked at better
than -9 mb, it will give good and faithfull service 20 years long.
-It needs absolutly to be baked each time it has seen atomspheric
pressure, to remove water vapor which limits its pumping cabability, as
in each vacuum sytem. A lite bake is processed at 150-250 °C, a much
stronger bakeout is done at 300°C. Above 300°C (up to 450 - 700°C)
magnets must be removed, but this is more a refurbishment procedure than
a maintenance one.

A aspect which is less known, at maybe this is your problem, is that
hydrocarbons may paralyse the pumping process. Under the ion current of
the pump and the e-beam of a TEM/SEM, one may polymerise them,
generating a wide familly of carbon products. These can be a real poison
for a ion pump. It's a known issue that one cannot put a ion pump on a
vaccum vessel fororganics evaporation (only diff, turbo or cryo). One
see always with a mass analyser a strong outgazing of CH4, CO, CO2 and
much heavier spices, at the starting or at the shutt off of the HV of
the pump, but in these cases much more. We have all seen the same
problem with Penning gauges, which are a modified design of the ion pump
(measuring without pumping, or pumping without measuring, different
design and material choice !).

In the case of a TEM/SEM, one have diff pumps, more or less good traped,
rotary vane pumps, more or les good traped too, and in your case,
"carbon" samples, which outgas carbon spices. Do you have a LN2 trap
near your sample stage ? Is a column vane between the sample stage and
the gun ? What is the "normal" vaccum in the gun, and is it measured by
a gauge, or the ion pump current ? This last point can give false
diagnostic : one think the pump isn't good anymore, and the vacuum level
is low, and in fact one have a good vacumm, but a wrong measuremnt,
distored by the leakage current of the pump. And one changes the pump !
In that case, the real point to verify is how does the vacumm go down,
dynamically, compared with the "normal" state.

I've more experience with ion pumps on clean UHV vessels than on TEMs,
but our TEM (Topcon 02B, with Lab6) has the first pump, which begin to
be now a bit tired after 15 years of work. Of coarse, we work on
materials, not on biological samples.

Hope it helps


J. Faerber
IPCMS-GSI
(Institut de Physique et Chimie des Matériaux de Strasbourg
Groupe Surface et Interfaces)
23, rue de Loess ; BP43
67034 Strasbourg CEDEX 2
France

Tel 00 33(0)3 88 10 71 01
Fax 00 33(0)3 88 10 72 48
E-mail Jacques.Faerber-at-ipcms.u-strasbg.fr



nizets2-at-yahoo.com a écrit :
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} Dear listers,
}
} We just changed the IGP pump of the gun chamber only 4 years after the installation of our Tecnai G20. This change was advised by a FEI engineer.
} We do not even have 400 working hours on this machine and I wondered if it was normal that we already have to change the pump.
} We work mainly with ultrathin sections of biological probes embedded in Epon. They are pretty contaminated with carbon, as evidenced by light circles remaining on the sections after even a very short illumination time (I am usually working at 120 kV, LaB6). I am wondering if this carbon contamination, evaporated by the electron beam, is not at least partly responsible for the dirtiness of the pumps (the pump of the column is bigger than the one for the gun, which would explain why it was not so dirty). If this is the case, perhaps a plasma cleaner would not only be a convenience for me but could bring a financial advantage for my boss (I know you see what I mean ;-)).
} What would be the cost of a plasma cleaner?
} What is your opinion on the question? Do you think that a plasma cleaner would increase the lifetime of the IGPs?
}
} Best regards,
}
} Stephane
}
}
} ____________________________________________________________________________________
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From: kjmorris-at-well.ox.ac.uk
Date: Thu, 31 Jan 2008 04:48:27 -0600
Subject: [Microscopy] TEM - negative scanners

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Hi Vachik,

Avoid the 9950F at all costs (I have one at home, and a few years ago it was
the best available but the Twain ScanGear software is absolute rubbish - it
can't even scan negatives to A4 and refuses to scan if film isn't in the
holders, ie. an unusual size). Plus it has lower resolution than the Epson
V750 pro - as does the older Epson 4990 so avoid that one as well.

The present best of the flatbed scanner bunch for large negatives and under
£1,000 (assuming you don't want to go to £10,000+) is the £600 Epson V750
Pro. We use it here to scan slide tissue sections as well as TEM negatives -
it's scan detail is noticeably better than our Nikon 1x objective and it has
far more even illumination (removing the microscope condenser for the 1x
objective makes microscope illumination very uneven). Naturally go to a 4x
or above objective and the microscope then to wins hands down - but if you
want general overviews of a tissue section the Epson V750 is fast and built
to scan flat things. Scans of film negatives are generally better in the
supplied holders (as the height of the film is right for focus).

In the rush to digital, film scanners are becoming a niche area, so we are
lucky there's still a few decent choices at under £1,000 - plus these cheap
scanners knock the socks off far more expensive scanners produced in the
late 1990s (in terms of image quality/resolution rather than ultimate build
quality anyway).

TEM negatives should last 500 years correctly archived so most users scan at
around 1,200 dpi for working copies rather than trying to archive images
scanned at the full 6,400 dpi resolution where the image size is massive
enough to be impractical for PC archiving (actually scanning at 3,200 dpi
with the V750 often produces similar detail to 6,400 dpi with most film, but
that’s still a very large image size in TIF). Don't throw away the B&W TEM
film after scanning, it should last up to 100 times longer than any
CD-RW/DVD-RW disk.

So have a look at the V750 Pro - it has better optics and is a more
versatile scanner than it's sibling V700 - although other extras like colour
targets are more related to colour balance for scanning colour film, but
worth having none the less. It scans up to an A4 negative, plus it can scan
in A4 reflective mode as well, and the twain Scan software is pretty good.
Only downside is the flimsy film holders - some buy new/spare ones* or have
their workshop build something suitable if they are scanning film all day.

I can send you a copy of my article on the subject of scanning film [RMS
InFocus & Microscopy Now] if you are interested.

Independent V750 review (as a colour film slide scanner)
http://www.photo-i.co.uk/index.html
http://www.photo-i.co.uk/Reviews/interactive/Epson%20V750/page_1.htm

*e.g. Doug Fishers film holders
http://www.betterscanning.com/
http://www.photo-i.co.uk/Reviews/interactive/Epson%204870/DF_holder/MF.htm
but may not suite TEM film sizes

Keith

--------------------------------------------------------------------------
Dr keith J. Morris
Molecular Cytogenetics and Microscopy Core
Laboratory 00/069 and 00/070
The Wellcome Trust Centre for Human Genetics
Roosevelt Drive
Oxford
OX3 7BN
United Kingdom
Telephone: +44 (0)1865 287568
Email: kjmorris-at-well.ox.ac.uk
Web-pages: http://www.well.ox.ac.uk/cytogenetics/



-----Original Message-----
X-from: vhacopian-at-wellesley.edu [mailto:vhacopian-at-wellesley.edu]
Sent: 30 January 2008 13:48
To: kjmorris-at-well.ox.ac.uk

I wish to purchase a flatbed scanner for TEM negatives. I have received
recommendations for the Canon 9950F and the Epson V750-M. The former may
no longer be available, as it is not listed on the Canon web site--only
the 8800F is. Any suggestions would be welcome and highly appreciated.
Vachik Hacopian


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From: nwwhite-at-babcock.com
Date: Thu, 31 Jan 2008 07:32:42 -0600
Subject: [Microscopy] viaWWW: vacuum problems JEOL JSM5600LV SEM

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hello Lee,

The first step is to discover if the problem is related to poor ultimate
vacuum or a bad gauge/controller. I have an independent vacuum gauge
installed on my SEM for just this purpose.

Woody



Woody White, Electron Microscopist
Babcock & Wicox
Technical Services Group
Lynchburg, VA


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Sent: Wednesday, January 30, 2008 5:51 PM
To: White, Woody N.

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Email: hadden-at-wingate.edu
Name: Lee Hadden

Organization: Wingate University

Title-Subject: [Filtered] vacuum problems JEOL JSM5600LV SEM

Question: Our JEOL 5600lv SEM does not attain operating vacuum. It goes
through the PRE-EVAC and into the EVAC modes in normal time frame, but
remains in EVAC, never going to READY for specimen observation. Any
ideas for fixing the problem? Cooling water temp and flow rate OK as
are DP temp and oil. The column will hold a vacuum for weeks + even with
the SEM off.

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From: smalinskas-at-yahoo.com
Date: Thu, 31 Jan 2008 07:46:25 -0600
Subject: [Microscopy] Re: viaWWW: vacuum problems JEOL JSM5600LV SEM

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Lee,

Our unit (JEOL JSM 5800LV) had an identical problem.
It would reach full vacuum, but not switch over to HT
READY. This problem came all of a sudden; it didn't
drift into the problem with pump times creeping into
longer intervals. The fix for our unit was to adjust
certain set points.

Our unit is under full service contract, so it was the
manufacturer's service tech that repaired our problem.
The fix was mentioned in the report... "adjusted TP 1
& 2 set points, TP1 set to 2.754, TP2 set to 1.584".
I don't know what that specifically means, nor whether
your unit has the same vacuum design. Maybe some of
this information can help you.

Stu Smalinskas, P.E.
SKF
Plymouth, Michigan
(734) 414-6862
--- hadden-at-wingate.edu wrote:

} Name: Lee Hadden
}
} Organization: Wingate University
}
} Title-Subject: [Filtered] vacuum problems JEOL
} JSM5600LV SEM
}
} Question: Our JEOL 5600lv SEM does not attain
} operating vacuum. It goes through the PRE-EVAC and
} into the EVAC modes in normal time frame, but
} remains in EVAC, never going to READY for specimen
} observation. Any ideas for fixing the problem?
} Cooling water temp and flow rate OK as are DP temp
} and oil. The column will hold a vacuum for weeks +
} even with the SEM off.
}


____________________________________________________________________________________
Looking for last minute shopping deals?
Find them fast with Yahoo! Search. http://tools.search.yahoo.com/newsearch/category.php?category=shopping

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From: Elliott-at-arizona.edu
Date: Thu, 31 Jan 2008 10:06:30 -0600
Subject: [Microscopy] TEM - negative scanners

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

I agree about the V750 pro being the current best in that price range.
David


On Jan 31, 2008, at 3:52 AM, kjmorris-at-well.ox.ac.uk wrote:

}
}
}
} ----------------------------------------------------------------------
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} The Microscopy ListServer -- CoSponsor: The Microscopy Society of
} America
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} MicroscopyListserver
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} ----------------------------------------------------------------------
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}
} Hi Vachik,
}
} Avoid the 9950F at all costs (I have one at home, and a few years
} ago it was
} the best available but the Twain ScanGear software is absolute
} rubbish - it
} can't even scan negatives to A4 and refuses to scan if film isn't
} in the
} holders, ie. an unusual size). Plus it has lower resolution than
} the Epson
} V750 pro - as does the older Epson 4990 so avoid that one as well.
}
} The present best of the flatbed scanner bunch for large negatives
} and under
} £1,000 (assuming you don't want to go to £10,000+) is the £600
} Epson V750
} Pro. We use it here to scan slide tissue sections as well as TEM
} negatives -
} it's scan detail is noticeably better than our Nikon 1x objective
} and it has
} far more even illumination (removing the microscope condenser for
} the 1x
} objective makes microscope illumination very uneven). Naturally go
} to a 4x
} or above objective and the microscope then to wins hands down - but
} if you
} want general overviews of a tissue section the Epson V750 is fast
} and built
} to scan flat things. Scans of film negatives are generally better
} in the
} supplied holders (as the height of the film is right for focus).
}
} In the rush to digital, film scanners are becoming a niche area, so
} we are
} lucky there's still a few decent choices at under £1,000 - plus
} these cheap
} scanners knock the socks off far more expensive scanners produced
} in the
} late 1990s (in terms of image quality/resolution rather than
} ultimate build
} quality anyway).
}
} TEM negatives should last 500 years correctly archived so most
} users scan at
} around 1,200 dpi for working copies rather than trying to archive
} images
} scanned at the full 6,400 dpi resolution where the image size is
} massive
} enough to be impractical for PC archiving (actually scanning at
} 3,200 dpi
} with the V750 often produces similar detail to 6,400 dpi with most
} film, but
} that’s still a very large image size in TIF). Don't throw away the
} B&W TEM
} film after scanning, it should last up to 100 times longer than any
} CD-RW/DVD-RW disk.
}
} So have a look at the V750 Pro - it has better optics and is a more
} versatile scanner than it's sibling V700 - although other extras
} like colour
} targets are more related to colour balance for scanning colour
} film, but
} worth having none the less. It scans up to an A4 negative, plus it
} can scan
} in A4 reflective mode as well, and the twain Scan software is
} pretty good.
} Only downside is the flimsy film holders - some buy new/spare ones*
} or have
} their workshop build something suitable if they are scanning film
} all day.
}
} I can send you a copy of my article on the subject of scanning film
} [RMS
} InFocus & Microscopy Now] if you are interested.
}
} Independent V750 review (as a colour film slide scanner)
} http://www.photo-i.co.uk/index.html
} http://www.photo-i.co.uk/Reviews/interactive/Epson%20V750/page_1.htm
}
} *e.g. Doug Fishers film holders
} http://www.betterscanning.com/
} http://www.photo-i.co.uk/Reviews/interactive/Epson%204870/DF_holder/
} MF.htm
} but may not suite TEM film sizes
}
} Keith
}
} ----------------------------------------------------------------------
} ----
} Dr keith J. Morris
} Molecular Cytogenetics and Microscopy Core
} Laboratory 00/069 and 00/070
} The Wellcome Trust Centre for Human Genetics
} Roosevelt Drive
} Oxford
} OX3 7BN
} United Kingdom
} Telephone: +44 (0)1865 287568
} Email: kjmorris-at-well.ox.ac.uk
} Web-pages: http://www.well.ox.ac.uk/cytogenetics/
}
}
}
} -----Original Message-----
} X-from: vhacopian-at-wellesley.edu [mailto:vhacopian-at-wellesley.edu]
} Sent: 30 January 2008 13:48
} To: kjmorris-at-well.ox.ac.uk
} Subject: [Microscopy] TEM - negative scanners
}
}
}
}
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} ----------------------------------------------------------------------
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}
} I wish to purchase a flatbed scanner for TEM negatives. I have
} received
} recommendations for the Canon 9950F and the Epson V750-M. The
} former may
} no longer be available, as it is not listed on the Canon web site--
} only
} the 8800F is. Any suggestions would be welcome and highly appreciated.
} Vachik Hacopian
}
}
} ==============================Original
} Headers==============================
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} 2008
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} 22, 23 -- From kjmorris-at-well.ox.ac.uk Thu Jan 31 04:48:26 2008
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} 22, 23 -- From: "Keith Morris" {kjmorris-at-well.ox.ac.uk}
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} 22, 23 -- Subject: RE: [Microscopy] TEM - negative scanners
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From: gary.m.brown-at-exxonmobil.com
Date: Thu, 31 Jan 2008 10:14:27 -0600
Subject: [Microscopy] viaWWW: 2 questions concerning microtomy of thin

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Sandra,

I agree with Jessica that you should use cryomicrotomy and collect dry
sections. This is a challenging technique but with practice you will find
it to be valuable. Microtome vendors and other training facilities offer
workshops on the cryomicrotomy.

In our lab we use a 'plastic chuck' for sectioning films at ambient and low
temperature. The chuck consists of a piece of plastic with approximate
dimensions of 4 mm x 7 mm x 3 mm (width x length x thickness). These
dimensions should be set to your personal preference and to fit your sample
and microtome chuck. Use a stiff plastic such as high density polyethylene
or polypropylene that will hold the sample tight but is not rigid or
inflexible. Using a sharp razor blade, bisect the 3 mm thickness, cutting
through nearly the full length of the plastic piece and leaving a couple of
millimeters of at the other end of the piece to hold the arms of the chuck
together. The end results is a Y-shaped piece of plastic (see diagram
below). To use the chuck, slide the film between the arms of the plastic
chuck leaving less than 1 mm exposed; the more film is exposed, the more
likely it is to move side-to-side during microtomy. Listers may contact me
off-line for a drawing of the chuck.

I recommend that you do not embed films in epoxy if at all possible. The
embedding medium, whatever it might be, only contributes to the difficulty
of cutting. The problem is that the film has several layers, each with
different cutting properties at low temperature; the problem is often even
worse at ambient temperature. Adding the embedding medium contributes
another medium that most probably has very different cutting properties
than any material in the film.

Disclaimer: The comments and opinions given above are those of the author
alone and do not represent any position of ExxonMobil Chemical Company.

Regards,

Gary M. Brown
Microscopy Specialist
ExxonMobil Chemical Company
Baytown Technology & Engineering - West
5200 Bayway Drive
Baytown, Texas 77520-2101
phone: 281 834 2387
fax: 281 834 2395
e-mail: Gary.M.Brown-at-ExxonMobil.com

"Our business in life is not to succeed, but to continue to fail in good
spirits." Robert Louis Stevenson






cervantes-at-bend
res.com
To
gary.m.brown-at-exxonmobil.com
01/30/08 07:40 cc
PM
Subject
[Microscopy] RE: viaWWW: 2 questions
Please respond concerning microtomy of thin films
to
cervantes-at-bend
res.com











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The Microscopy ListServer -- CoSponsor: The Microscopy Society of America


Sandra -

I also work with water soluble materials, and so often have to cut dry.
I have found that a diamond knife is preferable to glass (less "sticky"
so sections are easier to get off the knife surface), but that may be
something you want to experiment with. To transfer sections from the
knife to the grid, I use an eyelash probe (I buy mine from Ted Pella,
but people make them as well). It takes a little practice, but that is
what works best for me. I also use the probe to gently "flatten" the
sections onto the grid surface (I use 300 mesh Copper grids with Formvar
support film).

Diatome used to make a Cryo P diamond knife (don't know if they still
do) with a special platform that makes it easier to transfer sections.
This has been my favorite knife for dry-sectioning.

Sorry can't help with your second question, but hope this was useful.

Jessica

____________________
Jessica Cervantes
Bend Research Inc
64550 Research Rd
Bend, OR 97701
www.bendres.com





-----Original Message-----
X-from: sandra.gardner-at-xerox.com [mailto:sandra.gardner-at-xerox.com]
Sent: Wednesday, January 30, 2008 2:49 PM
To: Cervantes, Jessica

This Question/Comment was submitted to the Microscopy Listserver
using the WWW based Form at
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Email: sandra.gardner-at-xerox.com
Name: Sandra Gardner

Organization: Xerox Research Centre of Canada

Title-Subject: [Filtered] 2 questions concerning microtomy of thin films

Question: I have a multi layer film in which one of the layers is water
soluble. We want to cross section the sample for TEM to view the
various layers, each of which are less than 500nm thick. The total
thickness of the plastic substrate plus multilayer film is aprox.
500microns (the substate is aprox 300microns of this). I've embedded
the film in a epoxy resin for sectioning. I don't know how to go about
capturing thin sections ( {100nm) if I can't put water in the boat. I
could cut them dry, but again, I'm not sure how to transfer them to the
grid. I am using a Diatome diamond knife. Any suggestions would be
greatly appreciated.

Another question I have regards the use of tape as a support media for
cryo-sectioning. Many of our samples are films which I typically embed
in epoxy resin. We now have cryo-sectioning capabilities and i would
like to simply sandwich my film between tape and cryo cut thin films for
TEM analyses. Is there any tape which has good adhesion properties at
-120C and stand up well for TEM (glue does not interfere with sample)

Again, any direction is appreciated!

Login Host: 13.12.254.95
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From: mcauliff-at-umdnj.edu
Date: Thu, 31 Jan 2008 10:15:49 -0600
Subject: [Microscopy] Re: TEM - negative scanners

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Greetings all:

As I have suggested in the past, a digital camera can be used to
copy TEM negatives (or any larger format film). I put my negatives,
emulsion side up, on a light box, mask off the unwanted light with heavy
black paper or cardboard, and photograph the negative with an older (4
years or so) Canon G3 camera mounted on a copy stand to insure
stability. Most better digital cameras will focus close enough to fill
the frame with the negative (3.25 x 4 inches). I download the images to
Photoshop and invert to a positive. This is much faster than using a
flatbed scanner. The quality is fine for most applications. If you must
have higher quality for publication or making mural size prints, take
the negatives to a shop that has a drum scanner.

Geoff
vhacopian-at-wellesley.edu wrote:
} ----------------------------------------------------------------------------
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of America
} To Subscribe/Unsubscribe -- http://www.microscopy.com/MicroscopyListserver
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} I wish to purchase a flatbed scanner for TEM negatives. I have received
} recommendations for the Canon 9950F and the Epson V750-M. The former may
} no longer be available, as it is not listed on the Canon web site--only
} the 8800F is. Any suggestions would be welcome and highly appreciated.
} Vachik Hacopian
}
}
}
}
--
--
**********************************************
Geoff McAuliffe, Ph.D.
Neuroscience and Cell Biology
Robert Wood Johnson Medical School
675 Hoes Lane, Piscataway, NJ 08854
voice: (732)-235-4583
mcauliff-at-umdnj.edu
**********************************************



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5, 28 -- To: vhacopian-at-wellesley.edu, microscopy-at-microscopy.com
5, 28 -- Subject: Re: [Microscopy] TEM - negative scanners
5, 28 -- References: {200801301338.m0UDc1UX023749-at-ns.microscopy.com}
5, 28 -- In-reply-to: {200801301338.m0UDc1UX023749-at-ns.microscopy.com}
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From: mcauliff-at-umdnj.edu
Date: Thu, 31 Jan 2008 10:21:58 -0600
Subject: [Microscopy] Re: Can hardened fixed tissue be "softened" by Microwave

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi Tom:

I doubt if microwave exposure (cooking) will soften embalmed tissue.
You might try soaking the organ in water (tap water) for a week,
changing the water every day. There is good evidence that formalin-fixed
tissue can be "unfixed", at least to some extent, by prolonged washing
in water. Of course, it will depend on the composition of the embalming
fluid, the length of the exposure, etc.

Geoff


tbargar-at-unmc.edu wrote:
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} I've got a surgeon who is working with human livers that are very hard from
} the embalming process and he had heard that microwaving tissue may soften
} up the tissue and make it easier to cut. I'm going to let him use my
} Biowave and try different wattages. I have never heard of this effect
} before. Has anybody out there heard of or actually know if hardened fixed
} tissue can be softened by microwaves. Thanks, all help is appreciated.
}
} Tom Bargar
} University of Nebraska Medical Center
} Core Electron Microscopy Research Facility
} 986395 Nebraska Medical Center
} Omaha, NE 68198-6395
} 402-559-7347
} tbargar-at-unmc.edu
}
}
} ==============================Original Headers==============================
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--
--
**********************************************
Geoff McAuliffe, Ph.D.
Neuroscience and Cell Biology
Robert Wood Johnson Medical School
675 Hoes Lane, Piscataway, NJ 08854
voice: (732)-235-4583
mcauliff-at-umdnj.edu
**********************************************



==============================Original Headers==============================
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9, 29 -- Date: Thu, 31 Jan 2008 11:21:54 -0500
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9, 29 -- User-Agent: Thunderbird 2.0.0.9 (Windows/20071031)
9, 29 -- To: tbargar-at-unmc.edu, microscopy-at-microscopy.com
9, 29 -- Subject: Re: [Microscopy] Can hardened fixed tissue be "softened" by Microwave
9, 29 -- treatment?
9, 29 -- References: {200801291530.m0TFUBG4007543-at-ns.microscopy.com}
9, 29 -- In-reply-to: {200801291530.m0TFUBG4007543-at-ns.microscopy.com}
==============================End of - Headers==============================




From: beaurega-at-westol.com
Date: Thu, 31 Jan 2008 11:24:29 -0600
Subject: [Microscopy] Re: ion pump longevity

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi,

My IGP on my CM series TEM lasted 11-13 years. 4 years is quite short.,
IMO.

If you think you have carbon or hydrocarbon issues, have your serviceman
check the long column tubing liner just under the anode cap for a black
coating of residue that builds up on the liner's inner wall. There should
be a tool in the factory tool kit to remove this tubing liner. Look at the
amount of the deposit and the color. Ask the serviceman if that amount of
deposit seems normal or excessive. I would have a supply of 6-8 inch long
wooden "Q-tip swabs" and Pol polish handy for him.

HTH,

Paul

At 09:01 AM 1/30/08 -0600, you wrote:
}
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From: kjmorris-at-well.ox.ac.uk
Date: Thu, 31 Jan 2008 11:33:58 -0600
Subject: [Microscopy] Re: TEM - negative scanners

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi

A modern flatbed film scanner (e.g. the Epson V750) can scan a negative into
PhotoShop within a few minutes at 1,200 dpi - and there's no photo download
from camera to PC involved afterwards. At 6,400 dpi things do take a bit
longer, but that's well beyond the resolution of just about any camera prime
lens and indeed most colour slide film for that matter. If you compare a
camera macro image of a negative/slide to an Epson V750 film scan, it's no
contest - the Epson wins hands down.

TEM film has a higher theoretical resolution than 6,400 dpi but the
resulting TIF image file size from a slow 6,400 dpi V750 scan would be
highly prone to corruption if archived digitally on a PC anyway. You can
easily use 3,200 dpi to 'enlarge' selected areas of the negative though.
Plus we don't need Digital ICE scratch removal, which is the main process
that markedly slows down film scan speeds [but it can introduce artifacts
and affect detail, and anyway it isn't available for B&W film].

Besides, any process that passes an image back through another set of optics
will always further degrade that image. You should use a 8-10x inspection
magnifier and a light box to compare the scanned image with the original
film - the difference in resolution is small but clearly visible. Whatever
scanner is used, some detail is lost (just as detail was lost when the
original view was captured). Plus you really need to get the film/specimen
height and flatness right on a flatbed scanner, normally this means using
the supplied film holder (if the films at the wrong height from the platen
the scan image can be out of focus).

You do always get an apparent large reduction in shadow detail with a
pro-sumer V750 type flat bed scanner with colour slide film (shadows look
far too black), but the detail is actually still there and you can bring it
right back to the correct level of brightness using Photoshop's
'shadow/highlight' command. This quickly restores the shadow detail to the
scanned image. You can use PhotoShop's 'unsharp mask' [not much] to add back
a bit of sharpness at 100% mag as well. Always look at the original film
using a light box and 8-10x magnifier to ensure you get this post-scan
processing just right if that’s important to you.

The Epson 750 Pro produces image scans of comparable (if not
indistinguishable) quality to those of an £10k Hasselblad Imacon Flextight
848 semi-drum scanner - granted at far lower scan speeds. Besides 100 TEM
film scans using a Hasselblad in your Reprographics department would cost
you more than an Epson V750 pro anyway.

Keith


--------------------------------------------------------------------------
Dr keith J. Morris
Molecular Cytogenetics and Microscopy Core
Laboratory 00/069 and 00/070
The Wellcome Trust Centre for Human Genetics
Roosevelt Drive
Oxford
OX3 7BN
United Kingdom
Telephone: +44 (0)1865 287568
Email: kjmorris-at-well.ox.ac.uk
Web-pages: http://www.well.ox.ac.uk/cytogenetics/

-----Original Message-----
X-from: mcauliff-at-umdnj.edu [mailto:mcauliff-at-umdnj.edu]
Sent: 31 January 2008 16:23
To: kjmorris-at-well.ox.ac.uk

Greetings all:

As I have suggested in the past, a digital camera can be used to
copy TEM negatives (or any larger format film). I put my negatives,
emulsion side up, on a light box, mask off the unwanted light with heavy
black paper or cardboard, and photograph the negative with an older (4
years or so) Canon G3 camera mounted on a copy stand to insure
stability. Most better digital cameras will focus close enough to fill
the frame with the negative (3.25 x 4 inches). I download the images to
Photoshop and invert to a positive. This is much faster than using a
flatbed scanner. The quality is fine for most applications. If you must
have higher quality for publication or making mural size prints, take
the negatives to a shop that has a drum scanner.

Geoff
vhacopian-at-wellesley.edu wrote:
}
----------------------------------------------------------------------------
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of America
} To Subscribe/Unsubscribe --
http://www.microscopy.com/MicroscopyListserver
} On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
}
----------------------------------------------------------------------------
}
} I wish to purchase a flatbed scanner for TEM negatives. I have received
} recommendations for the Canon 9950F and the Epson V750-M. The former may
} no longer be available, as it is not listed on the Canon web site--only
} the 8800F is. Any suggestions would be welcome and highly appreciated.
} Vachik Hacopian
}
}
}
}
--
--
**********************************************
Geoff McAuliffe, Ph.D.
Neuroscience and Cell Biology
Robert Wood Johnson Medical School
675 Hoes Lane, Piscataway, NJ 08854
voice: (732)-235-4583
mcauliff-at-umdnj.edu
**********************************************



==============================Original Headers==============================
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5, 28 -- Date: Thu, 31 Jan 2008 11:15:44 -0500
5, 28 -- From: Geoff McAuliffe {mcauliff-at-umdnj.edu}
5, 28 -- User-Agent: Thunderbird 2.0.0.9 (Windows/20071031)
5, 28 -- To: vhacopian-at-wellesley.edu, microscopy-at-microscopy.com
5, 28 -- Subject: Re: [Microscopy] TEM - negative scanners
5, 28 -- References: {200801301338.m0UDc1UX023749-at-ns.microscopy.com}
5, 28 -- In-reply-to: {200801301338.m0UDc1UX023749-at-ns.microscopy.com}
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==============================Original Headers==============================
21, 23 -- From kjmorris-at-well.ox.ac.uk Thu Jan 31 11:33:56 2008
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21, 23 -- From: "Keith Morris" {kjmorris-at-well.ox.ac.uk}
21, 23 -- To: {Microscopy-at-Microscopy.Com}
21, 23 -- References: {200801311623.m0VGN5t8018582-at-ns.microscopy.com}
21, 23 -- Subject: RE: [Microscopy] Re: TEM - negative scanners
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From: bozzola-at-siu.edu
Date: Thu, 31 Jan 2008 14:46:18 -0600
Subject: [Microscopy] Re: Can hardened fixed tissue be "softened" by

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Vachik

I suspect that the Canon and Epson scanners will be more readily
available for negatives but it is still worth checking the specification
and prices of the Microtek i800 (semi pro) and i900 (pro). They both
have pretty good resolution and an excellect Dmax as well as using a
separate glassless drawer for negatives up to about 12 x 10 inches.

eg i800 review: "What's affordable about $400 list? How about a Dmax of
4.0, 48-bit color and 9600x4800 dpi optical resolution on a legal-sized
scanning bed with your choice of High-Speed USB 2.0 or FireWire ports?"
from http://www.imaging-resource.com/SCAN/MI8/MI8.HTM

The i900 is about twice the price but has an improved Dmax of 4.2.

I personally use the Microtek Scanmaker 8700 which still serves me well
but doesn't have the resolution or high Dmax of the two above.

Malcolm

Malcolm Haswell
e.m. unit
School of Health, Natural and Social Sciences
Fleming Building
University of Sunderland
Tyne & Wear
SR1 3SD
UK
e-mail: malcolm.haswell-at-sunderland.ac.uk






----- Original Message -----
X-from: vhacopian-at-wellesley.edu


In response to Tom Bargar's question,

I am not aware that microwaves can soften embalmed human liver
tissues. On the other hand, plant biologists often soak plant tissues
in glycerol to soften them for sectioning.

Check out the following article:

John C. Guenther and Frances Trail. 2005. The development and
differentiation of Gibberella zeae (anamorph: Fusarium graminearum)
during colonization of wheat. Mycologia, 97(1), 2005, pp. 229-237.

In this study, the authors did the following:

After a 24 h fixation, samples were placed in a solution of glycerol
and ethanol (1:1) for an additional 24 h to soften tissues for
sectioning.

They then further dehydrated the specimens in alcohol, embedded (in
paraffin, in this case) and sectioned as usual.
You might give it a try. Certainly, use the web to search for the use
of glycerine as a softener since I know it is used successfully.

Let us know what worked the best.

+++++++++++++++++++++++++++++++++++++++++++++++++++++++

John J. Bozzola, Ph.D., Director
Integrated Microscopy & Graphics Expertise (IMAGE)
Southern Illinois University
750 Communications Drive - MC 4402
Carbondale, IL 62901
Telephone: 618-453-3730

+++++++++++++++++++++++++++++++++++++++++++++++++++++++

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From: r-holdford-at-ti.com
Date: Thu, 31 Jan 2008 16:15:53 -0600
Subject: [Microscopy] 300mm wafer-capable SEM in North Texas?

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All: is there anyone in the north Texas area that has an SEM that will
take a 300mm (12-inch) wafer? I need to image the surface of a fully
processed, bumped wafer without coating it or breaking it.

--
~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~
Becky Holdford (r-holdford-at-ti.com)
972-995-2360
972-648-8743 (pager)
SC Packaging FA Development
Texas Instruments, Inc.
Dallas, TX
~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~


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From: johnf-at-geology.wisc.edu
Date: Thu, 31 Jan 2008 18:09:45 -0600
Subject: [Microscopy] EBSD workshop May 20-22

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The Microbeam Analysis Society is sponsoring a Technical Conference
on EBSD May 20-22 at the University of Wisconsin-Madison. The 3 day
workshop will start with a full day tutorial session for newcomers to
the technique. Student participation is being encouraged with 10 $500
scholarships. For more information and online registration materials,
go to www. microbeamanalysis.org. Space is limited so early
registration is strongly recommended.

John Fournelle
johnf-at-geology.wisc.edu

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From: mikroskop-at-gmail.com
Date: Thu, 31 Jan 2008 18:34:01 -0600
Subject: [Microscopy] viaWWW: magnification in CL images

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Email: mikroskop-at-gmail.com
Name: Jack Hietpas

Organization: Syracuse University

Title-Subject: [Filtered] magnification in CL images

Question: Hello: We have a JEOL 8600 Superprobe with what has been described as the "Poor man's" cathodoluminescence (CL) detector, which is simply a PMT inserted in the optical path of the probe's integrated light microscope. I have a very basic question concerning the system: where does the magnification of CL image come from? In addition why is the field of view the exact same as that in BSE or SEI? I find it hard to believe (perhaps incorrectly) that the magnification comes from the light microscope: the magnification is continuous as opposed to the fixed mag (focal length) of the light microscope and the mag range of the CL images is beyond the useful mag of the microscope. What am I missing?

-jh


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From: drix00-at-gmail.com
Date: Thu, 31 Jan 2008 19:11:44 -0600
Subject: [Microscopy] Re: viaWWW: magnification in CL images

Contents Retrieved from Microscopy Listserver Archives
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Hi Jack,

I don't know your exact setup, but my guess is that the signal from
the PMT is synchronized with the beam scanning on the sample. For each
position on the sample (pixel) the magnitude of the PMT is recorded as
the intensity on the image.
Just like a SE or BSE images.

Hendrix

On Jan 31, 2008 7:40 PM, {mikroskop-at-gmail.com} wrote:
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} Title-Subject: [Filtered] magnification in CL images
}
} Question: Hello: We have a JEOL 8600 Superprobe with what has been described as the "Poor man's" cathodoluminescence (CL) detector, which is simply a PMT inserted in the optical path of the probe's integrated light microscope. I have a very basic question concerning the system: where does the magnification of CL image come from? In addition why is the field of view the exact same as that in BSE or SEI? I find it hard to believe (perhaps incorrectly) that the magnification comes from the light microscope: the magnification is continuous as opposed to the fixed mag (focal length) of the light microscope and the mag range of the CL images is beyond the useful mag of the microscope. What am I missing?
}
} -jh
}
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From: dianavd-at-eye.usyd.edu.au
Date: Thu, 31 Jan 2008 20:43:57 -0600
Subject: [Microscopy] guinea pig fixation

Contents Retrieved from Microscopy Listserver Archives
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I have someone who wants to look at "changes" at the EM level caused
by experimental drugs, in guinea pig eyes. Hopefully he'll come up
with a more specific aim, but in the meantime does anyone have
experience fixing guinea pigs? I'll get him to perfuse the animals,
but would like to choose the best fixative. Any suggestions?

Thanks

Diana


Diana van Driel

Discipline of Ophthalmology
Sydney University
GPO Box 4337
Sydney, NSW
AUSTRALIA 2001

Phone 61 2 93827278
Mobile 0423 151614
FAX 61 2 93827318




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From: john.mardinly-at-intel.com
Date: Fri, 1 Feb 2008 14:48:13 -0600
Subject: [Microscopy] Re: ion pump longevity

Contents Retrieved from Microscopy Listserver Archives
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Hi all

The Microtek i800 scanner optical resolution is quoted at 4,800 dpi to the
Epsons V700/V750s 6,400 dpi - so it's probably on a par with the older 4,800
dpi Epsons and Canons - both of which were perfectly fine for TEM film scans
at 1,200 dpi anyway (other than Canon's Scangear being too stupid to notice
any film was on the platter).

Dmax is less important with B&W film (and this includes TEM) but is
essential resolving shadows with colour slides. Most modern scanners will
have a high enough DMax for B&W TEM film. The Hasselblad flextight has a
superb DMax and shadow detail in a colour slide was resolved very well, but
no better than the cheaper Epsons after post-processsing (the colour slide
film itself was the limiting factor really). The better resolution of the
8,000 dpi Hasselblad Flextight 848 drum scanner just picked out the detail
of the colour film grain better, and surprisingly didn't really get any
extra information from B&W TEM film (but I couldn't get to this scanner and
tweak it optimally for the TEM film - it was operated by the universities
Reprographics staff at £10 a scan.

Keith

--------------------------------------------------------------------------
Dr keith J. Morris
Molecular Cytogenetics and Microscopy Core
Laboratory 00/069 and 00/070
The Wellcome Trust Centre for Human Genetics
Roosevelt Drive
Oxford
OX3 7BN
United Kingdom
Telephone: +44 (0)1865 287568
Email: kjmorris-at-well.ox.ac.uk
Web-pages: http://www.well.ox.ac.uk/cytogenetics/


-----Original Message-----
X-from: malcolm.haswell-at-sunderland.ac.uk
[mailto:malcolm.haswell-at-sunderland.ac.uk]
Sent: 31 January 2008 17:46
To: kjmorris-at-well.ox.ac.uk

Vachik

I suspect that the Canon and Epson scanners will be more readily
available for negatives but it is still worth checking the specification
and prices of the Microtek i800 (semi pro) and i900 (pro). They both
have pretty good resolution and an excellect Dmax as well as using a
separate glassless drawer for negatives up to about 12 x 10 inches.

eg i800 review: "What's affordable about $400 list? How about a Dmax of
4.0, 48-bit color and 9600x4800 dpi optical resolution on a legal-sized
scanning bed with your choice of High-Speed USB 2.0 or FireWire ports?"
from http://www.imaging-resource.com/SCAN/MI8/MI8.HTM

The i900 is about twice the price but has an improved Dmax of 4.2.

I personally use the Microtek Scanmaker 8700 which still serves me well
but doesn't have the resolution or high Dmax of the two above.

Malcolm

Malcolm Haswell
e.m. unit
School of Health, Natural and Social Sciences
Fleming Building
University of Sunderland
Tyne & Wear
SR1 3SD
UK
e-mail: malcolm.haswell-at-sunderland.ac.uk






----- Original Message -----
X-from: vhacopian-at-wellesley.edu

Diana,

Years ago when we were perfusing mice and hamsters, we used a modified Krebs' Perfusion Buffer to flush the circulatory system, then fixed with a solution of 1% glut, 3% formaldehyde in PBS. Recipe for 100 mL Krebs is as follows (added in the order in which they appear):

0.17 g dextrose
0.02 g NaNO2
0.028 g heparin
2.0 mL 1M HEPES
1.0 g BSA
0.16 mL CaCl2 solution (0.147 g/mL)
pH 7.4

It takes about 40 mL to perfuse a mouse, so scale up accordingly.

Daryl Meyer

----- Original Message -----
X-from: dianavd-at-eye.usyd.edu.au


There are three little tricks for extending the life of ion pumps that
have not been mentioned yet that I thought I could contribute based on
years of experience with JEOL and Topcon TEM's:

1) The hammer. Yes, just smack the bajeezus out of the ion pump body
(not the magnet) with a hammer. The shock knocks most of the whiskers
and flakes loose. Do it with the emitter cold, because it will shock the
whole TEM. Put emphasis on a large number of mild whacks in every
direction of the pump housing. Keep the pump HV on, reading pump current
and you will see lots of little spikes as the whiskers and flakes get
dislodged. Wear hearing protection because you will need to do this for
about 20 minutes. When you stop seeing any spike in ion current with
hammer whacks, you are done.

2) Vent the system, pump it down, and restart the ion pump prematurely
with over current protection turned off. The pump should get hot. That's
basically a poor man's bake. It works.

3) Hi-pot. This is a technique where the service engineer brings in a
high current ~10KV power supply and connects it to the pump for about an
hour. The high voltage and high current blast all the whiskers and
flakes quite nicely. However, if you have never done this yourself, get
the service engineer to do it and be paranoid because it is VERY
DANGEROUS! If the standard power supply for ion pumps wasn't dangerous
enough, this is one that should treated with the greatest caution.

John Mardinly, Intel

This is not necessarily an opinion of Intel Corporation

-----Original Message-----
X-from: beaurega-at-westol.com [mailto:beaurega-at-westol.com]
Sent: Thursday, January 31, 2008 9:25 AM
To: Mardinly, John

Hi,

My IGP on my CM series TEM lasted 11-13 years. 4 years is quite short.,
IMO.

If you think you have carbon or hydrocarbon issues, have your serviceman
check the long column tubing liner just under the anode cap for a black
coating of residue that builds up on the liner's inner wall. There
should
be a tool in the factory tool kit to remove this tubing liner. Look at
the
amount of the deposit and the color. Ask the serviceman if that amount
of
deposit seems normal or excessive. I would have a supply of 6-8 inch
long
wooden "Q-tip swabs" and Pol polish handy for him.

HTH,

Paul

At 09:01 AM 1/30/08 -0600, you wrote:
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From: stephenson-at-impactanalytical.com
Date: Fri, 1 Feb 2008 15:49:18 -0600
Subject: [Microscopy] viaWWW: 2 questions concerning microtomy of thin films

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Greetings Sandra,

As usual Gary Brown is dead on with his comments. I agree that embedment is
generally best avoided in these multilayer applications. We have seen
swelling of the surface layer due to epoxy interaction as well, surprising
some real polymer gurus around here. His specimen holder sounds elegant - I
think I'll make one. We've taken a more down-and-dirty, and
semi-disposable, approach here that may be useful in some of your
applications.

We use some 15 mil (0.37 mm - thicker wouldn't hurt) high impact polystyrene
(HIPS) stock that was lying around to form a specimen support by cutting a
piece approximately twice as long as Gary cited, then folding it in half to
form an open envelope. The specimen is sandwiched between the folded ends
with the fold near the bottom of the chuck and the specimen just protruding
from the open end of the sandwich, also just above the microtome jaws.
Typically I will trim away the clamped envelope to form a little truncated
pyramid at the top and trim the sample to project just above, such that
almost all the sample is encased in the HIPS sandwich and the clamp. For
specimens that need more support (i.e. very thin films), the disposable
nature of this setup comes in handy. I trim away the entire assembly with
the specimen inside to form a mesa with HIPS and sample on the face (this is
especially helpful when cutting thick sections of multilayer films for light
microscopy). The HIPS sides of the pyramid are beveled as well to keep the
HIPS sectioning to a minimum. It is generally not a major problem to winnow
the sections of interest away from the sectioned support material, but make
sure you take the time to get to know the support material microstructure
intimately just in case! Good luck!

Yours,
Matt

Matthew Stephenson
Impact Analytical/MMI
1910 W. Saint Andrews Rd.
Midland, MI 48640
(989)832-5555 X506
stephenson-at-impactanalytical.com


-----Original Message-----
X-from: gary.m.brown-at-exxonmobil.com [mailto:gary.m.brown-at-exxonmobil.com]
Sent: Thursday, January 31, 2008 11:19 AM
To: stephenson-at-impactanalytical.com

Sandra,

I agree with Jessica that you should use cryomicrotomy and collect dry
sections. This is a challenging technique but with practice you will find
it to be valuable. Microtome vendors and other training facilities offer
workshops on the cryomicrotomy.

In our lab we use a 'plastic chuck' for sectioning films at ambient and low
temperature. The chuck consists of a piece of plastic with approximate
dimensions of 4 mm x 7 mm x 3 mm (width x length x thickness). These
dimensions should be set to your personal preference and to fit your sample
and microtome chuck. Use a stiff plastic such as high density polyethylene
or polypropylene that will hold the sample tight but is not rigid or
inflexible. Using a sharp razor blade, bisect the 3 mm thickness, cutting
through nearly the full length of the plastic piece and leaving a couple of
millimeters of at the other end of the piece to hold the arms of the chuck
together. The end results is a Y-shaped piece of plastic (see diagram
below). To use the chuck, slide the film between the arms of the plastic
chuck leaving less than 1 mm exposed; the more film is exposed, the more
likely it is to move side-to-side during microtomy. Listers may contact me
off-line for a drawing of the chuck.

I recommend that you do not embed films in epoxy if at all possible. The
embedding medium, whatever it might be, only contributes to the difficulty
of cutting. The problem is that the film has several layers, each with
different cutting properties at low temperature; the problem is often even
worse at ambient temperature. Adding the embedding medium contributes
another medium that most probably has very different cutting properties than
any material in the film.

Disclaimer: The comments and opinions given above are those of the author
alone and do not represent any position of ExxonMobil Chemical Company.

Regards,

Gary M. Brown
Microscopy Specialist
ExxonMobil Chemical Company
Baytown Technology & Engineering - West
5200 Bayway Drive
Baytown, Texas 77520-2101
phone: 281 834 2387
fax: 281 834 2395
e-mail: Gary.M.Brown-at-ExxonMobil.com

"Our business in life is not to succeed, but to continue to fail in good
spirits." Robert Louis Stevenson






cervantes-at-bend
res.com
To
gary.m.brown-at-exxonmobil.com
01/30/08 07:40 cc
PM
Subject
[Microscopy] RE: viaWWW: 2 questions
Please respond concerning microtomy of thin films
to
cervantes-at-bend
res.com











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The Microscopy ListServer -- CoSponsor: The Microscopy Society of America


Sandra -

I also work with water soluble materials, and so often have to cut dry.
I have found that a diamond knife is preferable to glass (less "sticky"
so sections are easier to get off the knife surface), but that may be
something you want to experiment with. To transfer sections from the knife
to the grid, I use an eyelash probe (I buy mine from Ted Pella, but people
make them as well). It takes a little practice, but that is what works best
for me. I also use the probe to gently "flatten" the sections onto the grid
surface (I use 300 mesh Copper grids with Formvar support film).

Diatome used to make a Cryo P diamond knife (don't know if they still
do) with a special platform that makes it easier to transfer sections.
This has been my favorite knife for dry-sectioning.

Sorry can't help with your second question, but hope this was useful.

Jessica

____________________
Jessica Cervantes
Bend Research Inc
64550 Research Rd
Bend, OR 97701
www.bendres.com





-----Original Message-----
X-from: sandra.gardner-at-xerox.com [mailto:sandra.gardner-at-xerox.com]
Sent: Wednesday, January 30, 2008 2:49 PM
To: Cervantes, Jessica

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Email: sandra.gardner-at-xerox.com
Name: Sandra Gardner

Organization: Xerox Research Centre of Canada

Title-Subject: [Filtered] 2 questions concerning microtomy of thin films

Question: I have a multi layer film in which one of the layers is water
soluble. We want to cross section the sample for TEM to view the various
layers, each of which are less than 500nm thick. The total thickness of the
plastic substrate plus multilayer film is aprox.
500microns (the substate is aprox 300microns of this). I've embedded the
film in a epoxy resin for sectioning. I don't know how to go about capturing
thin sections ( {100nm) if I can't put water in the boat. I could cut them
dry, but again, I'm not sure how to transfer them to the
grid. I am using a Diatome diamond knife. Any suggestions would be
greatly appreciated.

Another question I have regards the use of tape as a support media for
cryo-sectioning. Many of our samples are films which I typically embed in
epoxy resin. We now have cryo-sectioning capabilities and i would like to
simply sandwich my film between tape and cryo cut thin films for TEM
analyses. Is there any tape which has good adhesion properties at -120C and
stand up well for TEM (glue does not interfere with sample)

Again, any direction is appreciated!

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From: yashaa-at-hotmail.com
Date: Fri, 1 Feb 2008 16:49:12 -0600
Subject: [Microscopy] AskAMicroscopist: info on scanning transmission electron

Contents Retrieved from Microscopy Listserver Archives
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Below is the result of your feedback form (NJZFM-ultra-55). It was submitted by (yashaa-at-hotmail.com) from http://www.microscopy.com/Ask-A-Microscopist/Ask-A-Microscopist.html on Friday, February 1, 2008 at 16:42:01
---------------------------------------------------------------------------

Email: yashaa-at-hotmail.com
Name: Rasha ElBashir

Organization: Aachen university of applied science

Education: Graduate College

Location: Aachen, Germany

Question: I need some information for my study about the scanning transmission electron microscope (STEM), how does it work, what is it's principle and other basic information



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From: RCsencsits-at-lbl.gov
Date: Fri, 1 Feb 2008 17:18:08 -0600
Subject: [Microscopy] Re: AskAMicroscopist: info on scanning transmission electron

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Please Google "scanning transmission electron microscope" and within
the first 10 entries you will be off to a great start.

Roseann


On Feb 1, 2008, at 3:00 PM, yashaa-at-hotmail.com wrote:

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} Email: yashaa-at-hotmail.com
} Name: Rasha ElBashir
}
} Organization: Aachen university of applied science
}
} Education: Graduate College
}
} Location: Aachen, Germany
}
} Question: I need some information for my study about the scanning
} transmission electron microscope (STEM), how does it work, what is
} it's principle and other basic information
}
}


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From: bfostermme-at-sbcglobal.net
Date: Fri, 1 Feb 2008 17:34:38 -0600
Subject: [Microscopy] AskAMicroscopist: info on scanning

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

There is also a good overview on the FEI site. You can download "All you wanted to know about Electron MIcrosopy.... but didn't dare to ask."

Caveat: MME and The MIP have no commercial interest.

Hope this is helpful.
Barbara Foster, President

Microscopy/Microscopy Education
7101 Royal Glen Trail, Suite A
McKinney TX 75070
P: (972)924-5310
Skype: fostermme
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From: gary-at-gaugler.com
Date: Fri, 1 Feb 2008 17:52:57 -0600
Subject: [Microscopy] Re: AskAMicroscopist: info on scanning

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Different companies make their own flavor of STEM.
Here is a link to how Zeiss does it:

http://www.zeiss.com/C1256E4600307C70/EmbedTitelIntern/GEMINIMulti-ModeSTEMDetectionSystem/$File/GEMINI_multi-mode_STEM_detector_system.pdf

Mine is manual insertion and retraction of the solid state STEM
detector('s) diodes. The top side of the detector has four
diodes and another underneath. Switching amongst the
diodes provides BF and DF STEM.

Specimens are held in a standard 3mm diameter TEM grid and are typically
imaged at 30KV for highest resolution. Instead of a constant beam
of electrons flooding the specimen (like a TEM), the STEM does
electron beam scanning of the specimen. Quite a different
approach. Sometimes, very good and interesting results.

gary g.


At 02:52 PM 2/1/2008, you wrote:

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From: gary.m.brown-at-exxonmobil.com
Date: Fri, 1 Feb 2008 19:24:20 -0600
Subject: [Microscopy] viaWWW: 2 questions concerning microtomy of thin

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Matthew,

I learned about the plastic microtomy chuck from Lou Ban, a microscopist
who worked at Exxon Chemical some time ago. I've used it for +20 years
with success. Thanks, Lou.

You make good points regarding the specifics of use of the chuck during
microtomy. Your disposable chuck is ideal for the case in which a
cross-section of a thin film is needed for SEM/EDS. After cryo-sectioning
or cryo-facing (cryo-planing), the chuck/film assembly can be transferred
directly to the SEM for analysis.

We all have insight into what makes a better mousetrap, or in this case, a
microtomy chuck. The folks in our lab over the years used the chuck with
variations that fit their tastes and needs. Without folk's new ideas and
modifications of old ones, man wouldn't be where he is today.

Regards,

Gary M. Brown
Microscopy Specialist
ExxonMobil Chemical Company
Baytown Technology & Engineering - West
5200 Bayway Drive
Baytown, Texas 77520-2101
phone: 281 834 2387
fax: 281 834 2395
e-mail: Gary.M.Brown-at-ExxonMobil.com

"Our business in life is not to succeed, but to continue to fail in good
spirits." Robert Louis Stevenson






stephenson-at-imp
actanalytical.
com To
gary.m.brown-at-exxonmobil.com
cc
02/01/08 03:51
PM Subject
[Microscopy] RE: viaWWW: 2
questions concerning microtomy of
Please respond thi
to
stephenson-at-imp
actanalytical.
com











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Greetings Sandra,

As usual Gary Brown is dead on with his comments. I agree that embedment
is
generally best avoided in these multilayer applications. We have seen
swelling of the surface layer due to epoxy interaction as well, surprising
some real polymer gurus around here. His specimen holder sounds elegant -
I
think I'll make one. We've taken a more down-and-dirty, and
semi-disposable, approach here that may be useful in some of your
applications.

We use some 15 mil (0.37 mm - thicker wouldn't hurt) high impact
polystyrene
(HIPS) stock that was lying around to form a specimen support by cutting a
piece approximately twice as long as Gary cited, then folding it in half to
form an open envelope. The specimen is sandwiched between the folded ends
with the fold near the bottom of the chuck and the specimen just protruding
from the open end of the sandwich, also just above the microtome jaws.
Typically I will trim away the clamped envelope to form a little truncated
pyramid at the top and trim the sample to project just above, such that
almost all the sample is encased in the HIPS sandwich and the clamp. For
specimens that need more support (i.e. very thin films), the disposable
nature of this setup comes in handy. I trim away the entire assembly with
the specimen inside to form a mesa with HIPS and sample on the face (this
is
especially helpful when cutting thick sections of multilayer films for
light
microscopy). The HIPS sides of the pyramid are beveled as well to keep the
HIPS sectioning to a minimum. It is generally not a major problem to
winnow
the sections of interest away from the sectioned support material, but make
sure you take the time to get to know the support material microstructure
intimately just in case! Good luck!

Yours,
Matt

Matthew Stephenson
Impact Analytical/MMI
1910 W. Saint Andrews Rd.
Midland, MI 48640
(989)832-5555 X506
stephenson-at-impactanalytical.com


-----Original Message-----
X-from: gary.m.brown-at-exxonmobil.com [mailto:gary.m.brown-at-exxonmobil.com]
Sent: Thursday, January 31, 2008 11:19 AM
To: stephenson-at-impactanalytical.com


Sandra,

I agree with Jessica that you should use cryomicrotomy and collect dry
sections. This is a challenging technique but with practice you will find
it to be valuable. Microtome vendors and other training facilities offer
workshops on the cryomicrotomy.

In our lab we use a 'plastic chuck' for sectioning films at ambient and low
temperature. The chuck consists of a piece of plastic with approximate
dimensions of 4 mm x 7 mm x 3 mm (width x length x thickness). These
dimensions should be set to your personal preference and to fit your sample
and microtome chuck. Use a stiff plastic such as high density polyethylene
or polypropylene that will hold the sample tight but is not rigid or
inflexible. Using a sharp razor blade, bisect the 3 mm thickness, cutting
through nearly the full length of the plastic piece and leaving a couple of
millimeters of at the other end of the piece to hold the arms of the chuck
together. The end results is a Y-shaped piece of plastic (see diagram
below). To use the chuck, slide the film between the arms of the plastic
chuck leaving less than 1 mm exposed; the more film is exposed, the more
likely it is to move side-to-side during microtomy. Listers may contact me
off-line for a drawing of the chuck.

I recommend that you do not embed films in epoxy if at all possible. The
embedding medium, whatever it might be, only contributes to the difficulty
of cutting. The problem is that the film has several layers, each with
different cutting properties at low temperature; the problem is often even
worse at ambient temperature. Adding the embedding medium contributes
another medium that most probably has very different cutting properties
than
any material in the film.

Disclaimer: The comments and opinions given above are those of the author
alone and do not represent any position of ExxonMobil Chemical Company.

Regards,

Gary M. Brown
Microscopy Specialist
ExxonMobil Chemical Company
Baytown Technology & Engineering - West
5200 Bayway Drive
Baytown, Texas 77520-2101
phone: 281 834 2387
fax: 281 834 2395
e-mail: Gary.M.Brown-at-ExxonMobil.com

"Our business in life is not to succeed, but to continue to fail in good
spirits." Robert Louis Stevenson






cervantes-at-bend
res.com
To
gary.m.brown-at-exxonmobil.com
01/30/08 07:40 cc
PM
Subject
[Microscopy] RE: viaWWW: 2 questions
Please respond concerning microtomy of thin films
to
cervantes-at-bend
res.com











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Sandra -

I also work with water soluble materials, and so often have to cut dry.
I have found that a diamond knife is preferable to glass (less "sticky"
so sections are easier to get off the knife surface), but that may be
something you want to experiment with. To transfer sections from the knife
to the grid, I use an eyelash probe (I buy mine from Ted Pella, but people
make them as well). It takes a little practice, but that is what works
best
for me. I also use the probe to gently "flatten" the sections onto the
grid
surface (I use 300 mesh Copper grids with Formvar support film).

Diatome used to make a Cryo P diamond knife (don't know if they still
do) with a special platform that makes it easier to transfer sections.
This has been my favorite knife for dry-sectioning.

Sorry can't help with your second question, but hope this was useful.

Jessica

____________________
Jessica Cervantes
Bend Research Inc
64550 Research Rd
Bend, OR 97701
www.bendres.com





-----Original Message-----
X-from: sandra.gardner-at-xerox.com [mailto:sandra.gardner-at-xerox.com]
Sent: Wednesday, January 30, 2008 2:49 PM
To: Cervantes, Jessica

This Question/Comment was submitted to the Microscopy Listserver using the
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Email: sandra.gardner-at-xerox.com
Name: Sandra Gardner

Organization: Xerox Research Centre of Canada

Title-Subject: [Filtered] 2 questions concerning microtomy of thin films

Question: I have a multi layer film in which one of the layers is water
soluble. We want to cross section the sample for TEM to view the various
layers, each of which are less than 500nm thick. The total thickness of
the
plastic substrate plus multilayer film is aprox.
500microns (the substate is aprox 300microns of this). I've embedded the
film in a epoxy resin for sectioning. I don't know how to go about
capturing
thin sections ( {100nm) if I can't put water in the boat. I could cut them
dry, but again, I'm not sure how to transfer them to the
grid. I am using a Diatome diamond knife. Any suggestions would be
greatly appreciated.

Another question I have regards the use of tape as a support media for
cryo-sectioning. Many of our samples are films which I typically embed in
epoxy resin. We now have cryo-sectioning capabilities and i would like to
simply sandwich my film between tape and cryo cut thin films for TEM
analyses. Is there any tape which has good adhesion properties at -120C
and
stand up well for TEM (glue does not interfere with sample)

Again, any direction is appreciated!

Login Host: 13.12.254.95
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From: jacques.faerber-at-ipcms.u-strasbg.fr
Date: Mon, 4 Feb 2008 07:01:57 -0600
Subject: [Microscopy] Re: ion pump longevity more

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

And if things are so bad then on have to try some of the tricks
presented by John, here are two more :

-make a E-4 to E-6 O2 inlet in the pumpe while it's working. It may
refresh the Ti surface, by O2 ion reactive etching. Not easy to preform
on a microscope. One must have a leakvalve on the scope.

-make a vacuum in the 10E1 - 10 mbar range under air. Same effect
that former trick, but with more pressure and not pure oxygen. It's a DC
glow discharge. On a microscope it needs to put the vacuum control board
in manual mode, and to short some securities... The pump will warm up
too. One have together "baking" and ion etching.

Jacques


J. Faerber
IPCMS-GSI
(Institut de Physique et Chimie des Matériaux de Strasbourg
Groupe Surface et Interfaces)
23, rue de Loess ; BP43
67034 Strasbourg CEDEX 2
France

Tel 00 33(0)3 88 10 71 01
Fax 00 33(0)3 88 10 72 48
E-mail Jacques.Faerber-at-ipcms.u-strasbg.fr



john.mardinly-at-intel.com a écrit :
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} There are three little tricks for extending the life of ion pumps that
} have not been mentioned yet that I thought I could contribute based on
} years of experience with JEOL and Topcon TEM's:
}
} 1) The hammer. Yes, just smack the bajeezus out of the ion pump body
} (not the magnet) with a hammer. The shock knocks most of the whiskers
} and flakes loose. Do it with the emitter cold, because it will shock the
} whole TEM. Put emphasis on a large number of mild whacks in every
} direction of the pump housing. Keep the pump HV on, reading pump current
} and you will see lots of little spikes as the whiskers and flakes get
} dislodged. Wear hearing protection because you will need to do this for
} about 20 minutes. When you stop seeing any spike in ion current with
} hammer whacks, you are done.
}
} 2) Vent the system, pump it down, and restart the ion pump prematurely
} with over current protection turned off. The pump should get hot. That's
} basically a poor man's bake. It works.
}
} 3) Hi-pot. This is a technique where the service engineer brings in a
} high current ~10KV power supply and connects it to the pump for about an
} hour. The high voltage and high current blast all the whiskers and
} flakes quite nicely. However, if you have never done this yourself, get
} the service engineer to do it and be paranoid because it is VERY
} DANGEROUS! If the standard power supply for ion pumps wasn't dangerous
} enough, this is one that should treated with the greatest caution.
}
} John Mardinly, Intel
}
} This is not necessarily an opinion of Intel Corporation
}
} -----Original Message-----
} X-from: beaurega-at-westol.com [mailto:beaurega-at-westol.com]
} Sent: Thursday, January 31, 2008 9:25 AM
} To: Mardinly, John
} Subject: [Microscopy] Re: ion pump longevity
}
}
}
}
} ------------------------------------------------------------------------
} ----
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of
} America
} To Subscribe/Unsubscribe --
} http://www.microscopy.com/MicroscopyListserver
} On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} ------------------------------------------------------------------------
} ----
}
} Hi,
}
} My IGP on my CM series TEM lasted 11-13 years. 4 years is quite short.,
} IMO.
}
} If you think you have carbon or hydrocarbon issues, have your serviceman
} check the long column tubing liner just under the anode cap for a black
} coating of residue that builds up on the liner's inner wall. There
} should
} be a tool in the factory tool kit to remove this tubing liner. Look at
} the
} amount of the deposit and the color. Ask the serviceman if that amount
} of
} deposit seems normal or excessive. I would have a supply of 6-8 inch
} long
} wooden "Q-tip swabs" and Pol polish handy for him.
}
} HTH,
}
} Paul
}
} At 09:01 AM 1/30/08 -0600, you wrote:
}
} }
} } -----------------------------------------------------------------------
} }
} -----
}
} } The Microscopy ListServer -- CoSponsor: The Microscopy Society of
} }
} America
}
} } To Subscribe/Unsubscribe --
} }
} http://www.microscopy.com/MicroscopyListserver
}
} } On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} } -----------------------------------------------------------------------
} }
} -----
}
} } Dear listers,
} }
} } We just changed the IGP pump of the gun chamber only 4 years after the
} }
} installation of our Tecnai G20. This change was advised by a FEI
} engineer.
}
} } We do not even have 400 working hours on this machine and I wondered if
} }
} it
} was normal that we already have to change the pump.
}
} } We work mainly with ultrathin sections of biological probes embedded in
} }
} Epon. They are pretty contaminated with carbon, as evidenced by light
} circles remaining on the sections after even a very short illumination
} time
} (I am usually working at 120 kV, LaB6). I am wondering if this carbon
} contamination, evaporated by the electron beam, is not at least partly
} responsible for the dirtiness of the pumps (the pump of the column is
} bigger than the one for the gun, which would explain why it was not so
} dirty). If this is the case, perhaps a plasma cleaner would not only be
} a
} convenience for me but could bring a financial advantage for my boss (I
} know you see what I mean ;-)).
}
} } What would be the cost of a plasma cleaner?
} } What is your opinion on the question? Do you think that a plasma
} }
} cleaner
} would increase the lifetime of the IGPs?
}
} } Best regards,
} }
} } Stephane
} }
} }
} }
} }
} ________________________________________________________________________
} ____
} ________
}
} } Looking for last minute shopping deals?
} } Find them fast with Yahoo! Search.
} }
} http://tools.search.yahoo.com/newsearch/category.php?category=shopping
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} } ==============================Original
} }
} Headers==============================
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} } 6, 18 -- From nizets2-at-yahoo.com Wed Jan 30 09:00:54 2008
} } 6, 18 -- Received: from web37402.mail.mud.yahoo.com
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} 6, 16 -- Received: from mail.winbeam.com (mail.winbeam.com
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} 6, 16 -- From: Beaurega {beaurega-at-westol.com}
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} 19, 32 -- From john.mardinly-at-intel.com Fri Feb 1 14:48:11 2008
} 19, 32 -- Received: from mga11.intel.com (mga11.intel.com [192.55.52.93])
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} 19, 32 -- From: "Mardinly, John" {john.mardinly-at-intel.com}
} 19, 32 -- To: {beaurega-at-westol.com}
} 19, 32 -- Cc: {Microscopy-at-msa.microscopy.com}
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10, 29 -- From jacques.faerber-at-ipcms.u-strasbg.fr Mon Feb 4 07:01:57 2008
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From: jacques.faerber-at-ipcms.u-strasbg.fr
Date: Mon, 4 Feb 2008 08:10:14 -0600
Subject: [Microscopy] Re: ion pump longevity more Oups!

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Sorry for the oups!
I've forgotten the unit for the first trick, one has to read "E-4 to E-6
mbar O2 (oxygene)".
And a little "-" is missing in the second one " 10E-1 to 10 mbar".

It's not a good thing to answer to quickly !

And if things are so bad then on have to try some of the tricks
presented by John, here are two more :

-make a E-4 to E-6 mabr O2 inlet in the pump while it's working. It may
refresh the Ti surface, by O2 ion reactive etching. Not easy to perform
on a microscope. One must have a leakvalve on the scope.

-make a vacuum in the 10E-1 - 10 mbar range under air. Same effect
that former trick, but with more pressure and not pure oxygen. It's a DC
glow discharge. On a microscope it needs to put the vacuum control board
in manual mode, and to short some securities... The pump will warm up
too. One have together "baking" and ion etching.

Jacques


J. Faerber
IPCMS-GSI
(Institut de Physique et Chimie des Matériaux de Strasbourg
Groupe Surface et Interfaces)
23, rue de Loess ; BP43
67034 Strasbourg CEDEX 2
France

Tel 00 33(0)3 88 10 71 01
Fax 00 33(0)3 88 10 72 48
E-mail Jacques.Faerber-at-ipcms.u-strasbg.fr



john.mardinly-at-intel.com a écrit :
} ----------------------------------------------------------------------------
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of America
} To Subscribe/Unsubscribe -- http://www.microscopy.com/MicroscopyListserver
} On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} ----------------------------------------------------------------------------
}
}
} There are three little tricks for extending the life of ion pumps that
} have not been mentioned yet that I thought I could contribute based on
} years of experience with JEOL and Topcon TEM's:
}
} 1) The hammer. Yes, just smack the bajeezus out of the ion pump body
} (not the magnet) with a hammer. The shock knocks most of the whiskers
} and flakes loose. Do it with the emitter cold, because it will shock the
} whole TEM. Put emphasis on a large number of mild whacks in every
} direction of the pump housing. Keep the pump HV on, reading pump current
} and you will see lots of little spikes as the whiskers and flakes get
} dislodged. Wear hearing protection because you will need to do this for
} about 20 minutes. When you stop seeing any spike in ion current with
} hammer whacks, you are done.
}
} 2) Vent the system, pump it down, and restart the ion pump prematurely
} with over current protection turned off. The pump should get hot. That's
} basically a poor man's bake. It works.
}
} 3) Hi-pot. This is a technique where the service engineer brings in a
} high current ~10KV power supply and connects it to the pump for about an
} hour. The high voltage and high current blast all the whiskers and
} flakes quite nicely. However, if you have never done this yourself, get
} the service engineer to do it and be paranoid because it is VERY
} DANGEROUS! If the standard power supply for ion pumps wasn't dangerous
} enough, this is one that should treated with the greatest caution.
}
} John Mardinly, Intel
}
} This is not necessarily an opinion of Intel Corporation
}
} -----Original Message-----
} X-from: beaurega-at-westol.com [mailto:beaurega-at-westol.com]
} Sent: Thursday, January 31, 2008 9:25 AM
} To: Mardinly, John
} Subject: [Microscopy] Re: ion pump longevity
}
}
}
}
} ------------------------------------------------------------------------
} ----
} The Microscopy ListServer -- CoSponsor: The Microscopy Society of
} America
} To Subscribe/Unsubscribe --
} http://www.microscopy.com/MicroscopyListserver
} On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} ------------------------------------------------------------------------
} ----
}
} Hi,
}
} My IGP on my CM series TEM lasted 11-13 years. 4 years is quite short.,
} IMO.
}
} If you think you have carbon or hydrocarbon issues, have your serviceman
} check the long column tubing liner just under the anode cap for a black
} coating of residue that builds up on the liner's inner wall. There
} should
} be a tool in the factory tool kit to remove this tubing liner. Look at
} the
} amount of the deposit and the color. Ask the serviceman if that amount
} of
} deposit seems normal or excessive. I would have a supply of 6-8 inch
} long
} wooden "Q-tip swabs" and Pol polish handy for him.
}
} HTH,
}
} Paul
}
} At 09:01 AM 1/30/08 -0600, you wrote:
}
} }
} } -----------------------------------------------------------------------
} }
} -----
}
} } The Microscopy ListServer -- CoSponsor: The Microscopy Society of
} }
} America
}
} } To Subscribe/Unsubscribe --
} }
} http://www.microscopy.com/MicroscopyListserver
}
} } On-Line Help http://www.microscopy.com/MicroscopyListserver/FAQ.html
} } -----------------------------------------------------------------------
} }
} -----
}
} } Dear listers,
} }
} } We just changed the IGP pump of the gun chamber only 4 years after the
} }
} installation of our Tecnai G20. This change was advised by a FEI
} engineer.
}
} } We do not even have 400 working hours on this machine and I wondered if
} }
} it
} was normal that we already have to change the pump.
}
} } We work mainly with ultrathin sections of biological probes embedded in
} }
} Epon. They are pretty contaminated with carbon, as evidenced by light
} circles remaining on the sections after even a very short illumination
} time
} (I am usually working at 120 kV, LaB6). I am wondering if this carbon
} contamination, evaporated by the electron beam, is not at least partly
} responsible for the dirtiness of the pumps (the pump of the column is
} bigger than the one for the gun, which would explain why it was not so
} dirty). If this is the case, perhaps a plasma cleaner would not only be
} a
} convenience for me but could bring a financial advantage for my boss (I
} know you see what I mean ;-)).
}
} } What would be the cost of a plasma cleaner?
} } What is your opinion on the question? Do you think that a plasma
} }
} cleaner
} would increase the lifetime of the IGPs?
}
} } Best regards,
} }
} } Stephane
} }
} }
} }
} }
} ________________________________________________________________________
} ____
} ________
}
} } Looking for last minute shopping deals?
} } Find them fast with Yahoo! Search.
} }
} http://tools.search.yahoo.com/newsearch/category.php?category=shopping
}
} } ==============================Original
} }
} Headers==============================
}
} } 6, 18 -- From nizets2-at-yahoo.com Wed Jan 30 09:00:54 2008
} } 6, 18 -- Received: from web37402.mail.mud.yahoo.com
} }
} (web37402.mail.mud.yahoo.com [209.191.91.134])
}
} } 6, 18 -- by ns.microscopy.com (8.12.11.20060308/8.12.8) with SMTP
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} }
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}
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} } 6, 18 -- From: Stephane Nizet {nizets2-at-yahoo.com}
} } 6, 18 -- To: microscopy-at-microscopy.com
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} [64.84.96.10])
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} 6, 16 -- To: nizets2-at-yahoo.com, microscopy-at-microscopy.com
} 6, 16 -- From: Beaurega {beaurega-at-westol.com}
} 6, 16 -- Subject: Re: [Microscopy] ion pump longevity
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--
J. Faerber
IPCMS-GSI
(Institut de Physique et Chimie des Matériaux de Strasbourg
Groupe Surface et Interfaces)
23, rue de Loess ; BP43
67034 Strasbourg CEDEX 2
France

Tel 00 33(0)3 88 10 71 01
Fax 00 33(0)3 88 10 72 48
E-mail Jacques.Faerber-at-ipcms.u-strasbg.fr


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From: gary.m.brown-at-exxonmobil.com
Date: Mon, 4 Feb 2008 10:24:49 -0600
Subject: [Microscopy] Microtomy of polymer films and hard particles

Contents Retrieved from Microscopy Listserver Archives
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Dear Listers,

I was asked by a biological microscopist for information pertaining to
preparation and microtomy of polymer films and materials. Like many of us,
we are being asked to broaden our area of expertise into unfamiliar
territory. The following suggestions are based on guidance by several
other microscopists and much experience over the years. I don't claim to
be an expert, only a microscopist with a few proven tricks up my sleeve.
This is not a comprehensive or authoritative monograph, just friendly
advice. My hope is that this will cause a flurry of responses with
additional suggestions and ideas, questions (and answers) on preparation of
other sample types, and correction of any wrong statements by me.

Like biological microscopy, material science offers many challenges. The
broad spectrum of materials often requires only several key preparation and
microscopy tools and techniques. I would start with the materials that you
are presented with and worry about other potential challenges when they
arise. That said, there are several approaches to microtomy of materials
that are worth mentioning. As in every other aspect of microscopy, sample
preparation is absolutely essential.

Frankly, I learned most of the methods that I used by trial and error with
help from a few colleagues. I'm sure that a several if not many good
review papers and books deal with preparation techniques for
catalyst-related materials such as zeolites, aluminas, silicas, etc. These
are exceptionally important materials used to support catalyst species.
The microtome vendors can provide much insight into preparation of
materials for microscopy. Alternatively, other organizations such as
McCrone Associates may offer workshop.

Consider polishing if larger flat surfaces of hard materials are needed for
SEM analysis. Look for contract labs that will grind and polish your
samples until you have a sufficiently high sample volume that you need to
invest in grinding and polishing equipment.

Microtomy is the key to successful analysis of polymers. Several points
follow:
I generally try to avoid embedment. Exceptions to this are fibers,
fabrics and tiny particles that require rigid supports during
microtomy.
When embedment is unavoidable, try to match the hardness of the
medium to the sample as best possible.
IMPORTANT: Do not cure any embedding medium at a temperature
approaching the polymer melting point. If you don't know the melting
temperature, use an ambient curing epoxy such as EpoFix.
Polyolefins, a major class of polymers including polyethylene,
polypropylene, etc., require special care since their melting
temperatures can be as low as 40-50C or as high as 130-170C.
Embedded or not, section the polymer at a temperature below it's
glass transition temperature (Tg). When uncertain, lower the cutting
temperature to { -130C.
Cryo-section slowly since friction induced at higher rates can cause
heating of the polymer above it's Tg where it will soften and
plastically deform.

I use a standard approach to microtomy of hard materials like minerals and
catalyst supports. Low viscosity is an important requirement for any
embedding medium for small particles. I generally use LR White - hard
grade - without the accelerator because it is has very low viscosity, is
devoid of accelerator, is easy to use. The low viscosity allows it to
readily infiltrate most catalyst support particles giving good embedment.
Oven cure LR White at 80-90C for several hours in a nitrogen-purged oven.
On occasions, I will use EpoFix epoxy. Call your supplier of embedding
resins to find an epoxy:accelerator mixture that will give a hard block.
Cure at as high a temperature as is recommended by the manufacturer or your
supplier.
If the material is not in a finely powered form and grinding permits,
use a garnet mortar and pestle to finely divide the material.
Sprinkle the powder toward one end of a flat embedding mold. Take
care to have good density of particles in the mold but avoid piles or
clumps of catalyst since they may not be well infiltrated with the
embedding medium.
Degas the embedding medium in a vacuum to remove bubbles and absorbed
air. Epoxies and other higher viscosity embedding resins will take
longer to degas than lower viscosity resins like LR White.
Slowly layer the degassed embedding medium into the mold. Fully
cover the sample and fill the mold. Identify the sample with a small
paper label printed in pencil (ink runs when exposed to epoxy or LR
White) in the opposite end of the mold from the sample.
Place the mold plus catalyst into a vacuum and infiltrate for half an
hour or so. If the embedding resin begins to foam due to release of
air from within the powder, gently break vacuum several times until
the material is stable in the vacuum.
Heat cure in a nitrogen-purged oven for the required time.


Best regards,

Gary M. Brown
Microscopy Specialist
ExxonMobil Chemical Company
Baytown Technology & Engineering - West
5200 Bayway Drive
Baytown, Texas 77520-2101
phone: 281 834 2387
fax: 281 834 2395
e-mail: Gary.M.Brown-at-ExxonMobil.com

"Our business in life is not to succeed, but to continue to fail in good
spirits." Robert Louis Stevenson


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From: jekman-at-uiuc.edu
Date: Mon, 4 Feb 2008 14:11:24 -0600
Subject: [Microscopy] Job opening for Director of the Imaging Technology Group

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi All,

We have a job opening for Director of the Imaging Technology Group ITG has a
job opening for a new director.

The Beckman Institute at the University of Illinois, Urbana Champaign has a
position opening for one (1) Director, Imaging Technology Group (ITG). The
ITG's primary mission is to provide state-of-the-art imaging and
visualization resources for researchers at the Institute and the University
of Illinois. This mission is accomplished through two facilities: a
Microscopy Suite, and a Visualization, Media, and Imaging Laboratory. A
secondary mission of the ITG is to develop advanced technologies with an
emphasis on projects in remote and virtual instrumentation. The ITG Director
sets the vision for this group of approximately 25 staff members, writes
grants and directs special projects to support that vision, and conducts
daily management of the staff.

Read the announcement: http://www.itg.uiuc.edu/announcements/director.htm
and if you have questions, please contact jobs-at-beckman.uiuc.edu.

Cheers,

Jonathan M. Ekman
Imaging Technology Group
Beckman Institute for Advanced Science and Technology University of Illinois
at Urbana-Champaign
405 N. Mathews Avenue
Urbana, IL 61801 USA
Tel: 217-244-6292
Fax: 217-244-6219


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From: jquinn-at-www.matscieng.sunysb.edu
Date: Mon, 4 Feb 2008 16:53:26 -0600
Subject: [Microscopy] Microtomy of polymer films and hard particles

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html


Gary and folks -

I might add:

Get a good book such as Polymer Microscopy by Sawyer.

Polymer Microscopy, 2nd Edition
Linda Sawyer
David Grubb
Kluwer Academic Publishers
Hardbound, ISBN 0-412-60490-6
1995, 424 pages,
$333 US

regards,

Jim





From: jquinn-at-www.matscieng.sunysb.edu
Date: Mon, 4 Feb 2008 16:53:26 -0600
Subject: [Microscopy] Microtomy of polymer films and hard particles

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

==============================Original Headers==============================
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9, 12 -- Subject: re: Re: [Microscopy] Microtomy of polymer films and hard particles
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From: emer.ryan-at-dit.ie
Date: Tue, 5 Feb 2008 01:24:51 -0600
Subject: [Microscopy] viaWWW: grease for Sample exchange holder JEOL 8600 Superprobe

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Email: emer.ryan-at-dit.ie
Name: Emer Ryan

Organization: CREST DIT

Title-Subject: [Filtered] grease for Sample exchange holder JEOL 8600
Superprobe.

Question: Hello all,
I am using a JEOL JXA 8600 superprobe at the moment. Unfortunately,
the main microscopist is not available to help me with my query.
I am having a problem with sample exchange, as the rod doesn't slide
freely in and out of the exchange chamber.
I have cleaned/degreased the rod and re-greased again with the
lubricant that is there (no brand name available!) but after putting
the sample in place, the rod becomes black and sticks on removal.
As I am relatively new to microscopy - I would like some advice from
someone with a similar instrument regarding the correct grease to use
for this situation.

Thanks in advance.


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8, 11 -- From: emer.ryan-at-dit.ie (by way of MicroscopyListserver)
8, 11 -- Subject: viaWWW: grease for Sample exchange holder JEOL 8600 Superprobe
8, 11 -- Content-Type: text/plain; charset="us-ascii" ; format="flowed"
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From: yongli-at-mcb.harvard.edu
Date: Tue, 5 Feb 2008 01:25:17 -0600
Subject: [Microscopy] viaWWW: service for LKB 8800 Ultrotome III

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Email: yongli-at-mcb.harvard.edu
Name: Yong Li

Organization: Harvard University

Title-Subject: [Filtered] service for LKB 8800 Ultrotome III

Question: Hi,

There are a LKB 8800 Ultrotome III and its controller LKB 8802A in
the lab and they need to be serviced. But as LKB has disappeared, I
can't find any company to service on these two machines. Does anyone
know a company that does services on the LKB machines?

Thanks,

Yong Li



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From: jhuisken-at-gmail.com
Date: Tue, 5 Feb 2008 01:25:39 -0600
Subject: [Microscopy] viaWWW: Filter sets for Leica MZ16 F

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Email: jhuisken-at-gmail.com
Name: Jan Huisken

Organization: UCSF

Title-Subject: [Filtered] Filter sets for Leica MZ16 F

Question: Hi there,

We are planning on upgrading our Leica Stereoscopes (MZ16F) with new
filter sets. It turned out that Leica charges almost twice as much as
we would pay at Chroma for just the glass (ca. $1400 vs. $750). Is
anybody aware of a company that sells the empty filter holder so that
we can mount the filters ourselves?

Thanks,
Jan

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From: jacques.faerber-at-ipcms.u-strasbg.fr
Date: Tue, 5 Feb 2008 05:05:59 -0600
Subject: [Microscopy] Re: viaWWW: grease for Sample exchange holder JEOL 8600

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi

For a use such as the Jeol SEM's rod, I use Dow Corning High Vacuum
Grease. It's a silicon type grease. I do not use Apezon (L or M) vacuum
greases for dynamic use, only for static seals. Apiezon greases become
sticky, and hard. Silicon grease outgases a bit when fresh, but slides
very well. I suppose you may find other brands too (Nye, Monsanto or
others). Some people use a dropplet of dif pump oil (DC704/705), but it
needs to be cleaned and re-oiled more frequently.

The black traces may be dirt loosen by the freshly greased rod. In
case, clean it away with ethanol or aceton, and but a new set of (new)
grease. Wip away all grease which could accumulate at the end of the
rod. It will be only a dust trap !

I would not use an "unkown" brand of grease, unless you know it has be
given by the manufacturer of the intrument for that use.

Hope it helps

J. Faerber
IPCMS-GSI
(Institut de Physique et Chimie des Matériaux de Strasbourg
Groupe Surface et Interfaces)
23, rue de Loess ; BP43
67034 Strasbourg CEDEX 2
France

Tel 00 33(0)3 88 10 71 01
Fax 00 33(0)3 88 10 72 48
E-mail Jacques.Faerber-at-ipcms.u-strasbg.fr



emer.ryan-at-dit.ie a écrit :
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} Email: emer.ryan-at-dit.ie
} Name: Emer Ryan
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} Organization: CREST DIT
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} Title-Subject: [Filtered] grease for Sample exchange holder JEOL 8600
} Superprobe.
}
} Question: Hello all,
} I am using a JEOL JXA 8600 superprobe at the moment. Unfortunately,
} the main microscopist is not available to help me with my query.
} I am having a problem with sample exchange, as the rod doesn't slide
} freely in and out of the exchange chamber.
} I have cleaned/degreased the rod and re-greased again with the
} lubricant that is there (no brand name available!) but after putting
} the sample in place, the rod becomes black and sticks on removal.
} As I am relatively new to microscopy - I would like some advice from
} someone with a similar instrument regarding the correct grease to use
} for this situation.
}
} Thanks in advance.
}
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} ==============================Original Headers==============================
} 8, 11 -- From zaluzec-at-microscopy.com Tue Feb 5 01:24:51 2008
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} 8, 11 -- Subject: viaWWW: grease for Sample exchange holder JEOL 8600 Superprobe
} 8, 11 -- Content-Type: text/plain; charset="us-ascii" ; format="flowed"
} ==============================End of - Headers==============================
}

==============================Original Headers==============================
10, 30 -- From jacques.faerber-at-ipcms.u-strasbg.fr Tue Feb 5 05:05:59 2008
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From: eschumacher-at-mccrone.com
Date: Tue, 5 Feb 2008 09:15:13 -0600
Subject: [Microscopy] Short Course Announcement: TEM and SEM

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Greetings Fellow Microscopists,

The College of Microscopy, located in Westmont, IL, is offering the
following electron microscopy short courses:

March 25 to 27 - Transmission Electron Microscopy

March 31 to April 4 - Scanning Electron Microscopy

In addition to lectures, these courses emphasize hands-on training using
state of the art equipment. For further details and registration
information, please follow the link below.

www.collegeofmicroscopy.com



Elaine Schumacher
Senior Research Scientist
McCrone Associates, Inc.
850 Pasquinelli Drive
Westmont, IL 60559-5539 USA
630-887-7100 (tel)
630-887-7417 (fax)
E-mail: eschumacher-at-mccrone.com
Web Site: www.mccrone.com



==============================Original Headers==============================
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From: reinhard.rachel-at-biologie.uni-regensburg.de
Date: Tue, 5 Feb 2008 14:47:56 -0600
Subject: [Microscopy] ion pump longevity

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

As the topic is still discussed, here are a few sentences on our experience:

For an IGP pump, four years is short. 400 working hours far too short.
On our FEI CM12, after 17 years of use, always at 120 keV, about 48 weeks each year and } 40 hours each week, at least 10 or sometimes 15 different users per year, we only have the second IGP now in place, since about 3 or 4 years.
We have a TEM with a good vacuum, indeed.
Since end 1999, we have a slow-scan CCD - so we do not use film any more. So the TEM is always on and under vacuum, at least 360 days per year.
LaB6 filament: changed once in 3 years, only, although frequently used.
What we do: we always use LN2, every day. Every evening, we shut down the IGP, for four hours, during the time when the anti-contaminator is warming up. This is part of the software package we have (v.12.5).

This extends the lifetime of the IGP, we were told, by preventing the water, which was trapped at the anti-contaminator, from reaching the IGP. - This apparently helps to keep a good vacuum status, in general.

I have no financial interest in FEI - just a satisfied customer.
best regards - and hopefully always a good vacuum,
Reinhard

--

----------------------
PD Dr. Reinhard Rachel
Universitaet Regensburg
Centre for EM - NWF III -
-at-Institute for Anatomy
Universitaetsstr. 31
D-93053 Regensburg - Germany
tel +49 941 943 2837, 1720
fax +49 941 943 2868
mail reinhard.rachel-at-biologie.uni-r.de
office: VKL 3.1.29



==============================Original Headers==============================
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From: yuhong.wu-at-solvay.com
Date: Tue, 5 Feb 2008 23:22:03 -0600
Subject: [Microscopy] viaWWW: Polymer Failure Analysis book

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

This Question/Comment was submitted to the Microscopy Listserver
using the WWW based Form at http://www.microscopy.com/MLFormMail.html
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Email: yuhong.wu-at-solvay.com
Name: Yuhong Wu

Title-Subject: [Filtered] Polymer Failure Analysis book

Question: Dear All, I wonder if any of you works on failure analysis
of polymers(parts, film/fibers, composites etc.). And if there is any
good book/reference on that. I have a few books that have sections of
fracture/failure/fractography of polymers, a book named
"Compositional and failure analysis of polymers", another book
(coming soon) "Fractography - Observing, Measuring and Interpreting
Fracture".

I wonder if I am missing other good ones.

Thanks!

Yuhong

Login Host: 63.250.179.198
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==============================Original Headers==============================
8, 11 -- From zaluzec-at-microscopy.com Tue Feb 5 23:22:03 2008
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8, 11 -- To: microscopy-at-microscopy.com
8, 11 -- From: yuhong.wu-at-solvay.com (by way of MicroscopyListserver)
8, 11 -- Subject: viaWWW: Polymer Failure Analysis book
8, 11 -- Content-Type: text/plain; charset="us-ascii" ; format="flowed"
==============================End of - Headers==============================




From: yuhong.wu-at-solvay.com
Date: Tue, 5 Feb 2008 23:22:07 -0600
Subject: [Microscopy] viaWWW: Polymer Failure Analysis book

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

This Question/Comment was submitted to the Microscopy Listserver
using the WWW based Form at http://www.microscopy.com/MLFormMail.html
---------------------------------------------------------------------------
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please copy both yuhong.wu-at-solvay.com as well as the MIcroscopy Listserver
---------------------------------------------------------------------------

Email: yuhong.wu-at-solvay.com
Name: Yuhong Wu

Title-Subject: [Filtered] Polymer Failure Analysis book

Question: Dear All, I wonder if any of you works on failure analysis
of polymers(parts, film/fibers, composites etc.). And if there is any
good book/reference on that. I have a few books that have sections of
fracture/failure/fractography of polymers, a book named
"Compositional and failure analysis of polymers", another book
(coming soon) "Fractography - Observing, Measuring and Interpreting
Fracture".

I wonder if I am missing other good ones.

Thanks!

Yuhong

Login Host: 63.250.179.198
---------------------------------------------------------------------------

==============================Original Headers==============================
8, 11 -- From zaluzec-at-microscopy.com Tue Feb 5 23:22:06 2008
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8, 11 -- To: microscopy-at-microscopy.com
8, 11 -- From: yuhong.wu-at-solvay.com (by way of MicroscopyListserver)
8, 11 -- Subject: viaWWW: Polymer Failure Analysis book
8, 11 -- Content-Type: text/plain; charset="us-ascii" ; format="flowed"
==============================End of - Headers==============================




From: petra.wahlbring-at-goodyear.com
Date: Wed, 6 Feb 2008 02:00:29 -0600
Subject: [Microscopy] viaWWW: Polymer Failure Analysis book

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html


Yuhong,

I have a book that covers all kinds of fiber fracture and damage, polymeric
and natural ones. It's an atlas with lots of images and descriptions of the
failure mode:

Atlas of fibre fracture and damage to textiles. Second Edition. Hearle J W
S, Lomas B & Cooke W D. Woodhead Publishing. ISBN 1 85573 319 6

Best regards,

Petra
__________________________________
Dr. Petra Wahlbring
Lead Engineer Analytical Test Lab
GTC*L
Colmar-Berg, Luxembourg
e-mail: petra.wahlbring-at-goodyear.com
Tel. +352 8199 3725
Fax. +352 8199 5643


- May Contain Confidential and/or Proprietary Information. May not be
copied or disseminated without the express written consent of The Goodyear
Tire & Rubber Company. -

__________________





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Email: yuhong.wu-at-solvay.com
Name: Yuhong Wu

Title-Subject: [Filtered] Polymer Failure Analysis book

Question: Dear All, I wonder if any of you works on failure analysis
of polymers(parts, film/fibers, composites etc.). And if there is any
good book/reference on that. I have a few books that have sections of
fracture/failure/fractography of polymers, a book named
"Compositional and failure analysis of polymers", another book
(coming soon) "Fractography - Observing, Measuring and Interpreting
Fracture".

I wonder if I am missing other good ones.

Thanks!

Yuhong

Login Host: 63.250.179.198
---------------------------------------------------------------------------

==============================Original
Headers==============================
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==============================Original Headers==============================
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From: andrea.nans-at-gmail.com
Date: Wed, 6 Feb 2008 10:18:44 -0600
Subject: [Microscopy] TEM Sample Prep- Red Cell Skeleton Spread

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Dear All,

I am trying to prepare stripped and spread red blood cell skeletons for
negative stain EM. Briefly it involves isolating red blood cells through
centrifugation, hypotonic lysis to remove the hemoglobin, Triton X-100
extraction, and sucrose density gradient centrifugation under high
salt conditions. This should yield the basic skeleton of the red blood cell
which contains actin, spectrin, and 4.1. I am following the protocol by Shen
et al (Ultrastructure of unit fragments of the skeleton of the human
erythrocyte membrane. J. Cell. Biol. 99:810-821).

The problem I am having is that the skeletons I am isolating are aggregating
on the grids, and I am not sure if it is a problem with my sample
preparation protocol, my stain, or the grids. I've tried different
support films (holey and
continuous, plastic and carbon) and different negative stains (UA and Ammonium
molybdate of different concentrations). The grids have been both
glow-discharged
and non-glow-discharged. Diluting the sample with buffer does not
remedy the problem.
Is there a chance my prep is aggregating in solution? Some protocols
add a little DTT
to their suspension so I will next experiment with that. If there is
anyone who has experience
preparing these skeletons, any pointers would be greatly appreciated. Thank
you.

Andrea Nans
Graduate Student
NYU Med Center

==============================Original Headers==============================
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From: PhillipsT-at-missouri.edu
Date: Wed, 6 Feb 2008 10:23:14 -0600
Subject: [Microscopy] Wacom tablets/touch-screen monitors

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

I am thinking about buying a Wacom Cintiq monitor/tablet so that I can
trace objects during on the screen for Photoshop operations (e.g., area
measurements using the Fovea Pro toolkit). I would welcome comments
from those using this approach about its ease and success rate. The 6 x
10 inch workspace monitor is ~$1000 while the 17 x 10 is ~$2000. Any
thoughts on the size of the tablet or the DTF vs. Cintiq models would
also be useful. Thanks, Tom

Thomas E. Phillips, Ph.D
Professor of Biological Sciences
Director, Molecular Cytology Core
2 Tucker Hall
University of Missouri
Columbia, MO 65211-7400
573-882-4712 (office)
573-882-0123 (fax)
phillipst-at-missouri.edu

http://www.biology.missouri.edu/faculty/phillips.html
http://www.biotech.missouri.edu/mcc/




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From: gary.m.brown-at-exxonmobil.com
Date: Wed, 6 Feb 2008 13:49:48 -0600
Subject: [Microscopy] Re: viaWWW: Polymer Failure Analysis book

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Yuhong,

Lothar Engel et al., An Atlas of Polymer Damage - Surface Examination by
Scanning Electron Microscope, Prentice-Hall, New Jersey (1981) has been
useful to me. It is not comprehensive but helped in understanding the
morphology of polyolefin failure as seen using optical, SEM and TEM.

Regards,


Disclaimer: The comments and opinions given above are those of the author
alone and do not represent any position of ExxonMobil Chemical Company.

Gary M. Brown
Microscopy Specialist
ExxonMobil Chemical Company
Baytown Technology & Engineering - West
5200 Bayway Drive
Baytown, Texas 77520-2101
phone: 281 834 2387
fax: 281 834 2395
e-mail: Gary.M.Brown-at-ExxonMobil.com

"Happiness equals reality minus expectations" Tom Magliozzi






yuhong.wu-at-solv
ay.com
To
gary.m.brown-at-exxonmobil.com
02/05/08 11:25 cc
PM
Subject
[Microscopy] viaWWW: Polymer Failure
Please respond Analysis book
to
yuhong.wu-at-solv
ay.com











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Email: yuhong.wu-at-solvay.com
Name: Yuhong Wu

Title-Subject: [Filtered] Polymer Failure Analysis book

Question: Dear All, I wonder if any of you works on failure analysis
of polymers(parts, film/fibers, composites etc.). And if there is any
good book/reference on that. I have a few books that have sections of
fracture/failure/fractography of polymers, a book named
"Compositional and failure analysis of polymers", another book
(coming soon) "Fractography - Observing, Measuring and Interpreting
Fracture".

I wonder if I am missing other good ones.

Thanks!

Yuhong

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From: mcaruso2-at-uiuc.edu
Date: Thu, 7 Feb 2008 02:26:55 -0600
Subject: [Microscopy] [Filtered] AskAMicroscopist: Stain for imaging amines in epoxy

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This Question was submitted to Ask-A-Microscopist by (mcaruso2-at-uiuc.edu)
from
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Email: mcaruso2-at-uiuc.edu
Name: Mary M Caruso

Organization: University of Illinois at Urbana-Champaign

Education: Graduate College

Location: Urbana, IL, USA

Title: Stain for imaging amines in epoxy resin

Question: Do you know of a stain for electron microscopy that is
functional group specific? We would like to add a stain or dye that
would tag amines in an epoxy matrix to show that some of them have
not completely reacted in the 3D polymer network. I tried ninhydrin
as a stain and can see the purple color appear on the surface of the
resin but imaging these were more difficult.
Thank you for your help.
~Mary

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From: kjmorris-at-well.ox.ac.uk
Date: Thu, 7 Feb 2008 04:36:05 -0600
Subject: [Microscopy] Wacom tablets/touch-screen monitors

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi Thomas,

We used MetaMorph back at UCL and I bought a small $100 Wacom Graphire
version 2 A5 Tablet for image editing and tracing regions. The pen with this
set was superior to the latest (cheaper) Graphire v4 as the buttons were
located further down the pen as a single rocker and using the buttons was
far easier - which really affects how nice it is to use the tablet. The old
style pen looked more like the far more expensive Intuos 3 style. We didn't
need any larger than the little A5 pad for drawing around images of
cells/tissue on 22 inch CRT screen (any photos/negatives were scanned into
the PC rather than placed under the tablet to trace over). I would be
interested to hear from any who found the larger A4/A3 Wacon Intuos useful
for tracing (we don't do 'graphics' with it at work, it's always just
tracing, although my kids use a Graphire 2 with Corel Painter X at home).

Initially the works Wacom Graphire 2 tablet was hardly used and I disliked
it as the pen (and Wacom mouse) was so poor for basic Windows chores.
However when I had hundreds of cells to trace the Wacom Graphire 2 pad came
into it's own and it really helped tracing speed and accuracy (I just
wouldn't use a mouse to trace now if the pad was available). That said you
need the PC optical mouse as well to use menus etc.., they work happily with
the pen, you just drop the pen into it's holder and take over the curser
with the optical mouse when you have finished tracing (the pen providing the
double click to complete the trace).

When an unknown user lost the Graphire Pen (it looks like a normal pen and
probably got thrown away) we bought a cheap Graphire 4 pad - but I was
really unhappy with the pen button locations and ended up paying £30 for a
replacement Graphire 2 pen and used that pad instead (may just be habit).
The graphire 4 was half the price of the Graphire 2 (which did include a
rather naf mouse). So I would be tempted to go upmarket beyond the $80
Graphire 4, and go for something like an Intuos - and we found the smaller
A5 size perfect to fit on the desktop with a MS Intellimouse mouse.

I think an A4 tablet might have taken up too much room, but we bought the
little A5 Graphire 2 on a tight budget to try it out and never felt the need
to upgrade. I think the Cintiq may be going over the top just to trace
objects (and you can use the Intuos pen with the Cintiq if you upgrade
later) - but if that's all someone ever does in the lab, why not. Personally
I like using my PC monitor with a space saving A5 Wacom pad (that’s the same
size as the mouse pad). Our old Magiscan image analyzer back in the late
1980s had a light pen for drawing on the CRT screen (push on the glass
screen to 'mouse click') for image editing and that worked really well
[largely as the Magiscan image editing software was so good], so an
expensive Cintiq should be very successful as well. I did look into light
pens but they are expensive and aren't so software/LCD screen friendly as
tablets.

Enlarging the object [Zoom/magnify] onscreen really helped with accurate
tracing, and metaMorph has a useful back untrace function if you slip too
far off target. Some software just zooms in the area where you tracing,
which can be useful (I think ImagePro Plus v4/5 [Bio-rad LaserPix] did that,
but I can't remember exactly).

So the very cheap A5 wacom tablet was a success for us for occasional
tracing of microscope images - nearly always for tracing around cells from
wide field phase contrast [transmission] optical microscope images, eg. For
cell extention/retraction studies during wound healing. Have you tried a
cheaper Wacom Intuos 3 tablet and are wanting to upgrade for some reason ?

Regards

Keith

--------------------------------------------------------------------------
Dr keith J. Morris
Molecular Cytogenetics and Microscopy Core
Laboratory 00/069 and 00/070
The Wellcome Trust Centre for Human Genetics
Roosevelt Drive
Oxford
OX3 7BN
United Kingdom
Telephone: +44 (0)1865 287568
Email: kjmorris-at-well.ox.ac.uk
Web-pages: http://www.well.ox.ac.uk/cytogenetics/



-----Original Message-----
X-from: PhillipsT-at-missouri.edu [mailto:PhillipsT-at-missouri.edu]
Sent: 06 February 2008 16:36
To: kjmorris-at-well.ox.ac.uk

I am thinking about buying a Wacom Cintiq monitor/tablet so that I can
trace objects during on the screen for Photoshop operations (e.g., area
measurements using the Fovea Pro toolkit). I would welcome comments
from those using this approach about its ease and success rate. The 6 x
10 inch workspace monitor is ~$1000 while the 17 x 10 is ~$2000. Any
thoughts on the size of the tablet or the DTF vs. Cintiq models would
also be useful. Thanks, Tom

Thomas E. Phillips, Ph.D
Professor of Biological Sciences
Director, Molecular Cytology Core
2 Tucker Hall
University of Missouri
Columbia, MO 65211-7400
573-882-4712 (office)
573-882-0123 (fax)
phillipst-at-missouri.edu

http://www.biology.missouri.edu/faculty/phillips.html
http://www.biotech.missouri.edu/mcc/




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From: tbargar-at-unmc.edu
Date: Thu, 7 Feb 2008 09:35:00 -0600
Subject: [Microscopy] looking for an Ultracut E control box

Contents Retrieved from Microscopy Listserver Archives
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I'm looking for a control box for my Ultracut E ultramicrotome. If anyone
has one they would like to sell please contact me. Thanks.

Tom Bargar
University of Nebraska Medical Center
Core Electron Microscopy Research Facility
986395 Nebraska Medical Center
Omaha, NE 68198-6395
402-559-7347
tbargar-at-unmc.edu


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From: Elliott-at-arizona.edu
Date: Thu, 7 Feb 2008 09:54:53 -0600
Subject: [Microscopy] Wacom tablets/touch-screen monitors

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html


On Feb 7, 2008, at 3:40 AM, kjmorris-at-well.ox.ac.uk wrote:

}
I have not used the Cintiq (I don't have that kind of money), but I
have been using the Wacom Intuos for years now. For tracing objects
it is fantastic. For use with photoshop it is great.
I have found an added benefit. Switching between the 'pen' and the
mouse has alleviated some of my carpal tunnel problems. The
improvement has been great enough I got one for home also.
Another advantage for me is that I now have a mouse with 5 buttons
that can be individually programed for different applications. I have
gotten very used to this convenience. It is hard to go back to the
one button Mac mouse :-) I find the Wacom mouse (I have only used it
on the larger tablets) to be very usable.

David
}
}
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}
} I am thinking about buying a Wacom Cintiq monitor/tablet so that I can
} trace objects during on the screen for Photoshop operations (e.g.,
} area
} measurements using the Fovea Pro toolkit). I would welcome comments
} from those using this approach about its ease and success rate. The
} 6 x
} 10 inch workspace monitor is ~$1000 while the 17 x 10 is ~$2000. Any
} thoughts on the size of the tablet or the DTF vs. Cintiq models would
} also be useful. Thanks, Tom
}
} Thomas E. Phillips, Ph.D
} Professor of Biological Sciences
} Director, Molecular Cytology Core
} 2 Tucker Hall
} University of Missouri
} Columbia, MO 65211-7400
} 573-882-4712 (office)
} 573-882-0123 (fax)
} phillipst-at-missouri.edu
}
} http://www.biology.missouri.edu/faculty/phillips.html
} http://www.biotech.missouri.edu/mcc/
}
}
}
}
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} Headers==============================
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} 6, 23 -- From: "Phillips, Thomas E." {PhillipsT-at-missouri.edu}
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} 25, 23 -- From kjmorris-at-well.ox.ac.uk Thu Feb 7 04:36:05 2008
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5, 22 -- From Elliott-at-arizona.edu Thu Feb 7 09:54:53 2008
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From: michael-at-shaffer.net
Date: Thu, 7 Feb 2008 10:06:34 -0600
Subject: [Microscopy] Short course announcement: SEM-platform image analysis

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Memorial University of Newfoundland, located in St. John's, is pleased to
announce a short course on "Mineral Liberation Analysis" this spring, May
12-14, as well as an advanced course May 15-16. The courses are aimed at
minerals industry professionals and attendance is limited. More information
can be found in the announcement broshure:
http://www.mun.ca/creait/maf/MUN_MLA_Short_Course_2008_2.pdf

... and at our Micro-analysis Facility's website:
http://www.mun.ca/creait/maf/index.php
and
http://www.mun.ca/creait/maf/mla.php

Briefly, "Mineral Liberation Analysis" (MLA) refers primarily to economic
minerals and quantifying the degree to which they're liberated (or locked)
relative to other non-economic minerals. However, these specific mineral
relationships are only a subset of mineral associations for which the MLA is
also quite capable of quantifying. Other applications include
point-counting to rare-phase searches. In the past, MLA instrumentation has
been employed primarily at minerals' industry research locations worldwide;
however, has recently found its way into university research in the last
several years.

"Mineral Liberation Analysis" is a software solution that automates the
SEM's BEI and stage, as well as integrates high-speed x-ray spectral
acquisition (e.g., dual Bruker SDD x-ray detectors). The software was
developed at the University of Queensland's Julius Kruttschnitt Mineral
Research Centre (JKMRC), which is now the technology transfer company JKTech
Pty Ltd:
http://www.jktech.com.au/Products_Services/MLA/index.htm

Genuinely, Michael Shaffer :o)
SEM-MLA Research Coordinator
INCO Innovation Ctr
Memorial University
230 Elizabeth Avenue
St. John's Newfoundland A1C5S7
(709) 737-6799 (Ofc & Msg)
(709) 737-6790 (SEM Lab)
(709) 737-6193 (FAX)
http://www.mun.ca/creait/maf/


==============================Original Headers==============================
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6, 27 -- From: "michael shaffer" {michael-at-shaffer.net}
6, 27 -- To: "MSA Microscopy list" {Microscopy-at-microscopy.com}
6, 27 -- Subject: Short course announcement: SEM-platform image analysis
6, 27 -- Date: Thu, 7 Feb 2008 12:43:59 -0330
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From: vladislav_speransky-at-nih.gov
Date: Thu, 7 Feb 2008 11:57:56 -0600
Subject: [Microscopy] RE: Wacom tablets/touch-screen monitors

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hello Tom and Keith,

Keith, thanks for a thorough and informative post! And Tom, have you
actually been using a tablet already and now are considering an
upgrade to Cintiq? Or you haven't use either yet?

Anyway, I have just one comment to add now: that our hand (even my
clumsy one) seems to adjust very easily to any scaling when you trace
with a Wacom pen on your tablet while looking at the screen.
Seriously, I remember I was surprised at first. The hand learns
immediately and has no trouble following the outline, even if the
magnification on the screen is much higher. That means that bigger
tablet may not be better. Think about how exactly you will be using
it - setting on your desk in front of the monitor? or on your lap? on
your knee sitting with your legs crossed? We found Wacom's second
small size to be optimal. Bigger tablet can feel really bulky and
harder to balance; besides, there are those buttons on the tablet's
sides, and you won't be able to reach them as easy.

Vlad
________________________________________________
Vlad Speransky, Staff Scientist
Supramolecular Structure and Function Resource
National Institute of Biomedical Imaging and Bioengineering, NIH
13 South Dr, Rm. 3N17 MSC 5766
Bethesda, MD 20892
301 496-3989
vladislav_speransky-at-nih.gov


==============================Original Headers==============================
5, 22 -- From vladislav_speransky-at-nih.gov Thu Feb 7 11:57:56 2008
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5, 22 -- From: Vlad Speransky {vladislav_speransky-at-nih.gov}
5, 22 -- Subject: [Microscopy] RE: Wacom tablets/touch-screen monitors
5, 22 -- Date: Thu, 7 Feb 2008 12:57:37 -0500
5, 22 -- X-Mailer: Apple Mail (2.753)
==============================End of - Headers==============================




From: protrain-at-emcourses.com
Date: Thu, 7 Feb 2008 12:02:24 -0600
Subject: [Microscopy] Michaels Short Course announcement

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi

I have not complained before about course presentations but I feel Michaels
short course announcement goes beyond a course announcement and becomes a
sales presentation on a product.

Those of us who earn our crust through microscopy and selling a service take
great care not to step into a sales presentation situation; Michael I
believe has overstepped the mark?

Steve Chapman FRMS
Protrain for EM training & consultancy world wide
www.emcourses.com
Tel +44 1280 816512 Fax +44 1280 814007
Mobile +44 7711 606967



==============================Original Headers==============================
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From: PhillipsT-at-missouri.edu
Date: Thu, 7 Feb 2008 13:39:10 -0600
Subject: [Microscopy] RE: Wacom tablets/touch-screen monitors

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

I haven't used any type of tablet before. I must admit that reading
about them in some of the posts makes me wonder why I haven't. It is a
less expensive option. But some of the other posts are clearly extolling
the Cintiq which allows direct tracing on a near horizontal monitor. I
have used a mouse to trace 1000's of objects and I am fairly adept but I
know that I would have to be 10x faster tracing an object on a
photograph or, in this case, the monitor. I was mostly looking to hear
that this was as good as it seems on paper and it sounds like it should
be. I am definitely going to bite the bullet and buy either the small or
medium size monitor. I found the medium size one for 1900 and probably
will go with that. I will eventually post a comment about my results
once I get the new toy. I appreciate all the helpful comments. Tom



Thomas E. Phillips, Ph.D
Professor of Biological Sciences
Director, Molecular Cytology Core
2 Tucker Hall
University of Missouri
Columbia, MO 65211-7400
573-882-4712 (office)
573-882-0123 (fax)
phillipst-at-missouri.edu

http://www.biology.missouri.edu/faculty/phillips.html
http://www.biotech.missouri.edu/mcc/


-----Original Message-----
X-from: vladislav_speransky-at-nih.gov [mailto:vladislav_speransky-at-nih.gov]
Sent: Thursday, February 07, 2008 11:59 AM
To: Phillips, Thomas E.

Hello Tom and Keith,

Keith, thanks for a thorough and informative post! And Tom, have you
actually been using a tablet already and now are considering an
upgrade to Cintiq? Or you haven't use either yet?

Anyway, I have just one comment to add now: that our hand (even my
clumsy one) seems to adjust very easily to any scaling when you trace
with a Wacom pen on your tablet while looking at the screen.
Seriously, I remember I was surprised at first. The hand learns
immediately and has no trouble following the outline, even if the
magnification on the screen is much higher. That means that bigger
tablet may not be better. Think about how exactly you will be using
it - setting on your desk in front of the monitor? or on your lap? on
your knee sitting with your legs crossed? We found Wacom's second
small size to be optimal. Bigger tablet can feel really bulky and
harder to balance; besides, there are those buttons on the tablet's
sides, and you won't be able to reach them as easy.

Vlad
________________________________________________
Vlad Speransky, Staff Scientist
Supramolecular Structure and Function Resource
National Institute of Biomedical Imaging and Bioengineering, NIH
13 South Dr, Rm. 3N17 MSC 5766
Bethesda, MD 20892
301 496-3989
vladislav_speransky-at-nih.gov


==============================Original
Headers==============================
5, 22 -- From vladislav_speransky-at-nih.gov Thu Feb 7 11:57:56 2008
5, 22 -- Received: from nihrelayxway3.hub.nih.gov
(nihrelayxway3.hub.nih.gov [128.231.90.108])
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ESMTP id m17HvtHn002067
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11:57:55 -0600
5, 22 -- X-IronPortListener: NIH_Relay
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[128.231.217.77])
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format=flowed
5, 22 -- To: Microscopy-at-microscopy.com
5, 22 -- From: Vlad Speransky {vladislav_speransky-at-nih.gov}
5, 22 -- Subject: [Microscopy] RE: Wacom tablets/touch-screen monitors
5, 22 -- Date: Thu, 7 Feb 2008 12:57:37 -0500
5, 22 -- X-Mailer: Apple Mail (2.753)
==============================End of -
Headers==============================


==============================Original Headers==============================
16, 26 -- From PhillipsT-at-missouri.edu Thu Feb 7 13:39:10 2008
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16, 26 -- Subject: RE: [Microscopy] RE: Wacom tablets/touch-screen monitors
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16, 26 -- References: {200802071759.m17Hx6SO003334-at-ns.microscopy.com}
16, 26 -- From: "Phillips, Thomas E." {PhillipsT-at-missouri.edu}
16, 26 -- To: {vladislav_speransky-at-nih.gov}
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From: bozzola-at-siu.edu
Date: Thu, 7 Feb 2008 16:19:11 -0600
Subject: [Microscopy] LM: Wild M20 focus knob

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

We are attempting to repair a Wild M20 light microscope for a
colleague. The fine focus knob is no longer independently moveable
but is "fused" to the coarse focus. I believe the gearing mechanism
and associated metal parts need to be cleaned of polymerized
lubricant. I have disassembled the scope to gain access to the
gearing but cannot figure out how to remove the focus knobs to expose
the gearing. Does anyone know how this might be done? Thank you.
--
+++++++++++++++++++++++++++++++++++++++++++++++++++++++

John J. Bozzola, Ph.D., Director
Integrated Microscopy & Graphics Expertise (IMAGE)
Southern Illinois University
750 Communications Drive - MC 4402
Carbondale, IL 62901
Telephone: 618-453-3730

+++++++++++++++++++++++++++++++++++++++++++++++++++++++

==============================Original Headers==============================
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From: nizets2-at-yahoo.com
Date: Fri, 8 Feb 2008 02:15:33 -0600
Subject: [Microscopy] The mercury mystery

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi all!

No I don't present my last book, I just need your help to solve a mysterious peak in EDX ;-)
Here is the story:
A colleague was analysing a piece of zeolite in SEM with EDX (Tescan SEM, Oxford Instr. EDX). The specimen was sputter-coated with carbon and the HT was 20 keV (W filament).
I told her to try stick with a deadtime of about 20% and adjusted the parameters accordingly. At that moment we had the nice Al peak (1,49 keV), Si peak (1,74 keV) and a smaller but very clear Ca peak (3,69 keV). Happyness at its best.
Then I left her to have a cup of coffee...eer I mean to study a very difficult case and when I was back she said she found some mercury in the sample! (which is absolutely unexpected even as contaminant).
She had increased the spot size and had a deadtime of more than 70%!! And indeed she had a very tiny Hg peak at 2,19 keV! All others parameters being the same, when I decreased the spot size the Hg peak disappeared. This is obviously an artifact, but after reading the book from Goldstein, Newbury at al. I cannot find to which artifact belongs that Hg peak.
Any thought about it?

Best regards,

Stephane

PS: I will summarize the answers I got from my question about the IGP pump replacement soon


____________________________________________________________________________________
Never miss a thing. Make Yahoo your home page.
http://www.yahoo.com/r/hs

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From: A.A.Evans-at-Bradford.ac.uk
Date: Fri, 8 Feb 2008 02:34:52 -0600
Subject: [Microscopy] Wacom tablets/touch-screen monitors

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

I know it might sound silly, but why don't you have a go at making your own?
You already have the tablet.
http://www.bongofish.co.uk/wacom/wacom_pt1.html

I wasn't actually aware of the cintiq until the post on here, I've made do
with a regular tablet. After seeing the cintiq kit that wacom sell I think
it's superb, then I saw the price, and then I thought I'd bet I could make
my own. A couple of searches and I found this website; many people have
already done this with their own tablets and I'm about to have a bash too!

Hope this helps

-----Original Message-----
X-from: PhillipsT-at-missouri.edu [mailto:PhillipsT-at-missouri.edu]
Sent: 06 February 2008 16:34
To: a.a.evans-at-Bradford.ac.uk

I am thinking about buying a Wacom Cintiq monitor/tablet so that I can
trace objects during on the screen for Photoshop operations (e.g., area
measurements using the Fovea Pro toolkit). I would welcome comments
from those using this approach about its ease and success rate. The 6 x
10 inch workspace monitor is ~$1000 while the 17 x 10 is ~$2000. Any
thoughts on the size of the tablet or the DTF vs. Cintiq models would
also be useful. Thanks, Tom

Thomas E. Phillips, Ph.D
Professor of Biological Sciences
Director, Molecular Cytology Core
2 Tucker Hall
University of Missouri
Columbia, MO 65211-7400
573-882-4712 (office)
573-882-0123 (fax)
phillipst-at-missouri.edu

http://www.biology.missouri.edu/faculty/phillips.html
http://www.biotech.missouri.edu/mcc/




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From: kjmorris-at-well.ox.ac.uk
Date: Fri, 8 Feb 2008 03:41:49 -0600
Subject: [Microscopy] RE: Wacom tablets/touch-screen monitors

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Hi Tom,

I have to say, having got so used to a mouse, I find a Wacom standard mouse
pad A5 sized tablet and a stylus pen so intuitive as it is controlled just
like the mouse (even to the same scale of movement), but with far better
resolution - although I have to admit the little Wacom also meets my budget
requirements rather well and I'm less fussy about an perfect trace
(biological variation being rather greater than an exact outline). Plus
MetaMorph can undo [backtrace] so easily.

With a light pen on a 15inch CRT you are moving your arm around a lot more
(and back in the 1980/90s the screens were tough glass) - but I was
impressed compared the basic 1980s ball mouse - although the image editing
was hardware based back then not software, and so was lightening fast.

I wouldn't fancy a stylus on a modern soft fronted CRT screen - my
touchscreen PDAs and video camera screens are looking pretty manky after a
few years use with a stylus - as does my kids Nintendos, but they at least
have a plastic sticky screen protector (that looks naff with bubbles
everywhere). I find bending down to trace things a lot more fatiguing that
looking horizontally at a vertical PC monitor. Plus the A5 Wacom just hot
USB2 unplugs and goes in the drawer afterwards as desktop space is a premium
these days. Also Wacom tablets survive a hot cup of coffee and sandwich
crumbs with ease - and if they didn't they are also cheaper to replace
(stylues pens excepted, they are always getting lost). I guess I just don't
like tablet PCs really - handwriting is so last millennium - plus I want
plenty of raw power i.e. an imaging workstation desktop [laptops need not
apply].

I would be interested to get an update on the Cintiq if you get one - I'm
sure a lot of others on the list-server would as well.

Thanks for an interesting post.

Keith

--------------------------------------------------------------------------
Dr keith J. Morris
Molecular Cytogenetics and Microscopy Core
Laboratory 00/069 and 00/070
The Wellcome Trust Centre for Human Genetics
Roosevelt Drive
Oxford
OX3 7BN
United Kingdom
Telephone: +44 (0)1865 287568
Email: kjmorris-at-well.ox.ac.uk
Web-pages: http://www.well.ox.ac.uk/cytogenetics/

-----Original Message-----
X-from: PhillipsT-at-missouri.edu [mailto:PhillipsT-at-missouri.edu]
Sent: 07 February 2008 19:52
To: kjmorris-at-well.ox.ac.uk

I haven't used any type of tablet before. I must admit that reading
about them in some of the posts makes me wonder why I haven't. It is a
less expensive option. But some of the other posts are clearly extolling
the Cintiq which allows direct tracing on a near horizontal monitor. I
have used a mouse to trace 1000's of objects and I am fairly adept but I
know that I would have to be 10x faster tracing an object on a
photograph or, in this case, the monitor. I was mostly looking to hear
that this was as good as it seems on paper and it sounds like it should
be. I am definitely going to bite the bullet and buy either the small or
medium size monitor. I found the medium size one for 1900 and probably
will go with that. I will eventually post a comment about my results
once I get the new toy. I appreciate all the helpful comments. Tom



Thomas E. Phillips, Ph.D
Professor of Biological Sciences
Director, Molecular Cytology Core
2 Tucker Hall
University of Missouri
Columbia, MO 65211-7400
573-882-4712 (office)
573-882-0123 (fax)
phillipst-at-missouri.edu

http://www.biology.missouri.edu/faculty/phillips.html
http://www.biotech.missouri.edu/mcc/


-----Original Message-----
X-from: vladislav_speransky-at-nih.gov [mailto:vladislav_speransky-at-nih.gov]
Sent: Thursday, February 07, 2008 11:59 AM
To: Phillips, Thomas E.

Hello Tom and Keith,

Keith, thanks for a thorough and informative post! And Tom, have you
actually been using a tablet already and now are considering an
upgrade to Cintiq? Or you haven't use either yet?

Anyway, I have just one comment to add now: that our hand (even my
clumsy one) seems to adjust very easily to any scaling when you trace
with a Wacom pen on your tablet while looking at the screen.
Seriously, I remember I was surprised at first. The hand learns
immediately and has no trouble following the outline, even if the
magnification on the screen is much higher. That means that bigger
tablet may not be better. Think about how exactly you will be using
it - setting on your desk in front of the monitor? or on your lap? on
your knee sitting with your legs crossed? We found Wacom's second
small size to be optimal. Bigger tablet can feel really bulky and
harder to balance; besides, there are those buttons on the tablet's
sides, and you won't be able to reach them as easy.

Vlad
________________________________________________
Vlad Speransky, Staff Scientist
Supramolecular Structure and Function Resource
National Institute of Biomedical Imaging and Bioengineering, NIH
13 South Dr, Rm. 3N17 MSC 5766
Bethesda, MD 20892
301 496-3989
vladislav_speransky-at-nih.gov


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30, 22 -- From kjmorris-at-well.ox.ac.uk Fri Feb 8 03:41:41 2008
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From: kraftpiano-at-gmail.com
Date: Fri, 8 Feb 2008 07:28:27 -0600
Subject: [Microscopy] SEM Short Course recommendations.

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

I am planning my 2008 year professional development right now, and I
would like to take a short (but intensive) course in SEM imaging. I
would like to learn how to bring out better images, as well as some
sample preparation techniques for biological samples. I can get away
for up to a week for a course, possibly with return visits at a later
date for follow-up. If anyone has taken such a course, or offers one,
please send your comments to me off-list.

Thanks,

Justin A. Kraft

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From: nizets2-at-yahoo.com
Date:
Subject:

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

What
about
that
solution?

http://www.cs.cmu.edu/~johnny/projects/wii/

Watch
the
first
video,
it
is
amazing!

Best
regards,
Stephane

-----
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8,
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35, 19 -- From nizets2-at-yahoo.com Fri Feb 8 07:43:16 2008
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From: mcgeejj-at-kapl.gov
Date: Fri, 8 Feb 2008 08:22:47 -0600
Subject: [Microscopy] Open Position - Surface scientist for materials science applications

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Lockheed Martin- KAPL, Inc. has an open position for a surface scientist
(experienced in Auger / ESCA techniques). A brief description of the
job is given below. NOTE: US Citizenship REQUIRED.

The complete job announcement (Req ID 66233BR) can be found at the
Lockheed Martin career web site (LockheedMartin.com).

Jim McGee
************************************
James J. McGee
Materials Engineer, Test Operations
Lockheed Martin, KAPL, Inc.
Mail Bin 149
PO Box 1072
Schenectady, NY 12301-1072

Tel: 518-395-4612
Fax: 518-395-4340
email: mcgeejj-at-kapl.gov
************************************



Req ID 66233BR

Industry Job Title Materials Engineer Sr

Required skills: MS degree in the physical sciences (e.g. materials
science, chemistry, geology, solid state physics) or engineering, plus
hands-on training and/or experience operating scanning Auger electron
microscopy (SAM), Electron Spectroscopy for Chemical Analysis (ESCA),
and Secondary Ion Mass Spectrometry (SIMS).
Desired skills PhD degree in physical sciences with 5 years or more
experience in surface and microanalysis (SAM, ESCA, and SIMS) and
demonstrated problem solving experience in areas of metallurgy, alloy
testing/development, solid inorganic materials, and/or ceramics.
Previous experience and nuclear or radioactive materials, corrosion,
metallurgy, and ceramics is a also desirable.

Specific Job Description: Characterize the surfaces of materials to
support environmental testing and failure analysis of in-service
components. Utilize field-emission Auger electron microscopy and
imaging, ESCA spectroscopy and imaging, and SIMS. Execute data and image
processing (e.g. Target-Factor Analysis (TFA, PCA), curve fitting,
quantitative analysis, data assimilation, and reporting of results.
Participate in multidisciplinary, collaborative investigations and
team-oriented problem solving with other materials characterization
specialists and materials scientists/engineers using associated
analytical techniques (FEG-SEM, EBSD, EPMA, XRD, TEM, FTIR, Raman, FIB,
TOF-SIMS).

The major duties will be the use of advanced surface analytical
techniques to determine the microstructure and microchemistry of metals,
alloys, and ceramic materials. Ensure instrumentation is properly
maintained and in proper operating condition. Analyze and interpret data
and communicate results to sponsoring groups by oral and written
reports. Serve as part of research teams to design experiments that will
elucidate structure-composition-property-processing relationships. Stay
current in surface and microanalytical techniques and applications and
propose/implement new capabilities or characterization tools.




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From: stephenson-at-impactanalytical.com
Date: Fri, 8 Feb 2008 08:56:17 -0600
Subject: [Microscopy] The mercury mystery

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html


Greetings Stephane,

The math would fit for the escape of Al x-rays during the detection of Ca
(3.69 - 1.49). I wouldn't ordinarily expect that you would detect that sort
of an escape peak, but at 70 dead time, who knows...? When your colleague
cranked the dead time, did you also detect a new peak at 1.95, corresponding
to Ca minus Si? If your mystery peak is an escape peak, I would think you
would see this one as well.

Yours,
Matt

Matthew Stephenson
Impact Analytical/MMI
1910 W. Saint Andrews Rd.
Midland, MI 48640
(989)832-5555 X506
stephenson-at-impactanalytical.com
Visit Impact Analytical in Booth # 3305 at PittCon March 3rd - 7th

-----Original Message-----
X-from: nizets2-at-yahoo.com [mailto:nizets2-at-yahoo.com]
Sent: Friday, February 08, 2008 3:23 AM
To: stephenson-at-impactanalytical.com

Hi all!

No I don't present my last book, I just need your help to solve a mysterious
peak in EDX ;-) Here is the story:
A colleague was analysing a piece of zeolite in SEM with EDX (Tescan SEM,
Oxford Instr. EDX). The specimen was sputter-coated with carbon and the HT
was 20 keV (W filament).
I told her to try stick with a deadtime of about 20% and adjusted the
parameters accordingly. At that moment we had the nice Al peak (1,49 keV),
Si peak (1,74 keV) and a smaller but very clear Ca peak (3,69 keV).
Happyness at its best.
Then I left her to have a cup of coffee...eer I mean to study a very
difficult case and when I was back she said she found some mercury in the
sample! (which is absolutely unexpected even as contaminant).
She had increased the spot size and had a deadtime of more than 70%!! And
indeed she had a very tiny Hg peak at 2,19 keV! All others parameters being
the same, when I decreased the spot size the Hg peak disappeared. This is
obviously an artifact, but after reading the book from Goldstein, Newbury at
al. I cannot find to which artifact belongs that Hg peak.
Any thought about it?

Best regards,

Stephane

PS: I will summarize the answers I got from my question about the IGP pump
replacement soon



____________________________________________________________________________
________
Never miss a thing. Make Yahoo your home page.
http://www.yahoo.com/r/hs

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==============================Original Headers==============================
16, 26 -- From stephenson-at-impactanalytical.com Fri Feb 8 08:56:16 2008
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16, 26 -- Subject: RE: [Microscopy] The mercury mystery
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From: bharris-at-uoguelph.ca
Date: Fri, 8 Feb 2008 09:28:32 -0600
Subject: [Microscopy] TEM: Collagen in the Patella

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Good Morning: I have a potential project to compare the mechanical
properties of collagen in the kneecap with its structure and
arrangement. First I'm not sure this is a TEM project as another type
of microscopy might be better. Secondly I assume I would have to embed
and section the patella and could really use some help on the "how
to". If anyone has experience working with this material I would be
pleased to get some advice. Thanks bob harris

Guelph Regional Integrated Imaging Facility (GRIIF)
Transmission Electron Microscope Facility
Dept. of Molecular and Cell Biology
New Science Complex, 488 Gordon St.
University of Guelph
Guelph Ontario, Canada, N1G 2W1
Phone: 519-824-4120 X 56409
Fax: 519-837-1802




==============================Original Headers==============================
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From: albinab-at-ornl.gov
Date: Fri, 8 Feb 2008 14:48:18 -0600
Subject: [Microscopy] Postdoctoral position in Combined Scanning Transmission and Scanning

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Dear listers,
Below please find a description of a postdoctoral opportunity at Oak
Ridge National Laboratory. Feel free to post or forward to any qualified
candidates.

*Combined Scanning Transmission and Scanning Probe Microscopy of
Ferroelectrics*

*Materials Science and Technology Division *

*Oak Ridge National Laboratory *

*Oak Ridge, Tennessee *

*Project Description: *

The Materials Science and Technology Division at Oak Ridge National
Laboratory (ORNL) is seeking a candidate to fill a postdoctoral position
in the field of combined scanning transmission electron microscopy and
scanning probe microscopy of ferroelectric thin films. The position is
available immediately. This program takes advantage of ORNL’s suite of
advanced electron microscopes, including 4 aberration-corrected
instruments, as well as recently acquired (S)TEM/STM and (S)TEM/AFM
capabilities.

The successful applicant must demonstrate experience in electron
microscope operation, preferably FEI microscopes, as well as skills in
analysis and interpretation of microscopic and spectroscopic data. This
position provides an opportunity to join an experienced team working in
a highly collaborative environment on the projects ranging from
heterogeneous catalysis to oxide materials to semiconductors. Close
interactions with the scanning probe microscopy program at ORNL’s Center
for Nanophase Materials Sciences (CNMS) are anticipated.

*Qualifications: PhD degree required *

This position requires a Ph.D. in Materials Science, Physics, or related
field, with an emphasis on advanced TEM or STEM. Knowledge of oxide
crystal chemistry is a plus. Excellent oral and written communication
skills are required, and presentations and publication of scientific
results in peer-reviewed journals are expected. The applicant must have
the ability to work in a team and interact effectively with a broad
range of colleagues. Applicants cannot have received the most recent
degree more than five years prior to the date of application and must
complete all degree requirements before starting their appointment.

*How to Apply: *

Qualified applicants may apply online at https://www2.orau.gov/ORNL_POST/ .

All applicants will need to register before they can begin the online
application. For complete instructions, on how to apply, please see the
instructions at

http://www.orau.gov/orise/edu/ornl/ornl-pdpm/application.htm . When
applying for this position, please reference the position title and
number ORNL08-23-MSTD). Questions regarding the position can be directed
to Drs. Albina Y. Borisevich, albinab-at-ornl.gov
{mailto:albinab-at-ornl.gov} , Stephen J. Pennycook, pennycooksj-at-ornl.gov
{mailto:pennycooksj-at-ornl.gov} , and Sergei V. Kalinin, sergei2-at-ornl.gov
{mailto:sergei2-at-ornl.gov} . Applications will be accepted until the
position is filled. This appointment is offered through the ORNL
Postgraduate Research Participation Program and is administered by the
Oak Ridge Institute for Science and Education (ORISE). The program is
open to all qualified U.S. and non-U.S. citizens without regard to race,
color, age, religion, sex, national origin, physical or mental
disability, or status as a Vietnam-era veteran or disabled veteran.

--
--
Albina Y. Borisevich
R&D Associate
Electron Microscopy Group
Oak Ridge National Laboratory
Materials Science and Technology Division
PO Box 2008
Oak Ridge TN 37831-6031

http://stem.ornl.gov/

For express mail add: 1 Bethel Valley Road
phone: (865) 576-4060
fax: (865) 574-4143

==============================Original Headers==============================
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From: connellyps-at-nhlbi.nih.gov
Date: Fri, 8 Feb 2008 16:50:41 -0600
Subject: [Microscopy] Hotel for M&M

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Greetings,

I have gone on line today to reserve my room for M&M 2008 and I chose the
Double Tree Hotel. The rate for two was $125 instead of $119 as published
on the Microscopy web site (I challenged this). There were no rooms
available for Wed. and Thurs. at the discounted meeting rate. I inquired
about non-discount rooms, not wishing to pack up and move and they were
available at $165, if I remember correctly. Luckily the thrifty little voice
in my head spoke up and I was able to get a AAA discount and the cost was
$151 and $143.

The message from MSA was correct about the rooms going quickly!

Pat Connelly


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From: friess-at-limedion.de
Date: Fri, 8 Feb 2008 17:24:48 -0600
Subject: [Microscopy] \viaWWW: JEOL 6xxxF Series with the serial (RS232) interface

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Email: friess-at-limedion.de
Name: Frank Frieþ

Organization: LMI

Title-Subject: [Filtered] 6300F/6400F/6600F

Question: Hi,

is there someone here who is running a JEOL 6xxxF
Series with the serial (RS232) interface
activated ? If it can be read (and maybe even be
controled) some parameters like magnification,
voltage etc. by a connected computer system (e.g.
EDS) this would be an indicater that the serial
is working. (as I found out the interface was
often not activated when the devices were sold).
I would be happy to find someone with a working
RS232.

thanks in advance

Frank

Login Host: 84.173.145.245
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From: hanke-at-mee-inc.com
Date: Fri, 8 Feb 2008 18:05:12 -0600
Subject: [Microscopy] Re: viaWWW: Polymer Failure Analysis book

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

There are a few basic FA books on polymers out there. It seems that no
one book covers the topic sufficiently to be "the" reference. The book
you now have and the Engel book previously recommended are good. My
other favorites:
Failure of Plastics and Rubber Products by David Wright
Plastics Failure Analysis and Prevention, John Moalli (Editor)
Plastics Failure Guide by Myer Ezrin

--
Larry D. Hanke, P.E.
Materials Evaluation and Engineering, Inc.
Practical Solutions Through Technology and Innovation
http://www.mee-inc.com (763) 449-8870


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From: stefan.diller-at-t-online.de
Date: Mon, 11 Feb 2008 12:58:20 -0600
Subject: [Microscopy] FEI EM 208S problem

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Dear All,
has someone out there a procedure for opening up the column of a 1997 EM
208S at the specimen stage to get a jammed prep-holder out again?
Anything special to take care of?

Best regards,
Stefan



Aktuelles: "Die Ästhetik des Unsichtbaren" - Pflanzenoberflächen unter dem
Elektronenmikroskop
Siehe www.elektronenmikroskopie.info/ausstelllungen/wuerzburg
Mein Jahreskalender 2008 zum herunterladen und selbst ausdrucken im Format
DIN A3:
www.quantifoil.com/calendar_2008.pdf (38 MB)
Falls Sie Bilder daraus kommerziell verwenden möchten fragen Sie mich bitte
vorher...

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From: nizets2-at-yahoo.com
Date: Tue, 12 Feb 2008 05:01:35 -0600
Subject: [Microscopy] the mercury mystery solved!!

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Dear list,

Here is a summary of the different answers and finally what I think is the right one.
I want to thank everybody for their help, I received lots of answers, almost all different but all very interesting.

1) Hg may be an escape peak of Ca. However in my book, and as someone stated, this does not really fit well.
Ca (3,69) -1,74 (following my book) is not very near to 2,19 (Hg peak)

2) It is not a contamination, since this Hg peaks appears only at (too) high a deadtime. It clearly indicates an artifact.

3) One comment stated "It's the Ca peak (3.69) exciting the Al peak (1.49) leaving a 2.20 kV X-ray to exit the sample". I don't understand it!! (sorry)

3) The most reasonable answer is a pileup peak of O+Si. The 2 peaks are the 2 highest in the spectrum and their addition perfectly fits to the Hg peak. The person who proposed that solution seems to be experienced with this type of material and problem and this pileup does not seem so uncommon for high deadtimes.

I hope this can help others.

Best regards,
Stephane


____________________________________________________________________________________
Looking for last minute shopping deals?
Find them fast with Yahoo! Search. http://tools.search.yahoo.com/newsearch/category.php?category=shopping

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From: wesaia-at-iastate.edu
Date: Tue, 12 Feb 2008 09:15:24 -0600
Subject: [Microscopy] the mercury mystery solved!!

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

I concur with number 3. I strongly suspected O+Si was the explanation.
Since I hadn't seen it suggest as an answer, I threw some SiO2 into our
older SEM yesterday afternoon and collected spectra at 20%, 30%, and 60%
deadtime. I pasted the spectra and analytical results into a file which
you may find here (ftp://www.marl.iastate.edu/General/SiO2_with_Hg.pdf
). You can see the "Hg" peak increase with increasing deadtime. You can
also see the O+O and Si+Si sum peaks, but the "Hg" O+Si sum peak seems
to be the highest in this case.

The analytical results quantify the effect. The Hg mass fraction is
reported as 1.3, 1.7 and 6.8%. I did not push the exercise to lower
deadtimes. I also did not try tweaking our old Kevex pulse processor to
improve its pile-up rejection (for the record, the Kevex feeds an IXRF
Systems box). I should repeat this experiment on our newer EDS system
and see if it performs any better.

The moral of the story is that sum peaks are one of the main reasons
that deadtime needs to be limited. Also, just because you can't see a
peak (e.g., O or C) doesn't mean in can't pile up and appear in the
spectrum.

Warren Straszheim
Materials Analysis and Research Lab
Iowa State University

-----Original Message-----
X-from: nizets2-at-yahoo.com [mailto:nizets2-at-yahoo.com]
Sent: Tuesday, February 12, 2008 5:03 AM
To: wesaia-at-iastate.edu

Dear list,

Here is a summary of the different answers and finally what I think is
the right one.
I want to thank everybody for their help, I received lots of answers,
almost all different but all very interesting.

1) Hg may be an escape peak of Ca. However in my book, and as someone
stated, this does not really fit well.
Ca (3,69) -1,74 (following my book) is not very near to 2,19 (Hg peak)

2) It is not a contamination, since this Hg peaks appears only at (too)
high a deadtime. It clearly indicates an artifact.

3) One comment stated "It's the Ca peak (3.69) exciting the Al peak
(1.49) leaving a 2.20 kV X-ray to exit the sample". I don't understand
it!! (sorry)

3) The most reasonable answer is a pileup peak of O+Si. The 2 peaks are
the 2 highest in the spectrum and their addition perfectly fits to the
Hg peak. The person who proposed that solution seems to be experienced
with this type of material and problem and this pileup does not seem so
uncommon for high deadtimes.

I hope this can help others.

Best regards,
Stephane



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From: bigelow-at-umich.edu
Date: Tue, 12 Feb 2008 14:20:08 -0600
Subject: [Microscopy] RE: Vacuum Grease

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

You can find a fairly detailed description of various vacuum greases
in Sect. 10.12 (p.458) of my book 'Vacuum Methods in Electron
Microscopy' I would recommend one of the perfluorinated polyphenyl
ether greases Brayco 803 or Krytox LVP for most applications in
electron microscopy. These greases are excellent lubricants, and are
chemically inert (and so should not cause any corrosive reactions
with metal parts), and have vapor pressures in the 10^-10 Torr
range. However, I have recently learned of a grease called
Santovac-5GB that is based on the polyphenyl ether vacuum fluid
Santovac-5 which also has excellent properties (vapor pressure of 4 x
10^-10 Torr, stable up to 450 C, excellent as a lubricant, no
tendency to spread or bleed, etc.) and which might be equally good.
Some people prefer not to use the perfluorinated compounds in their
instruments, and so this might be a good alternative choice. You can
find a detailed description of both types of grease in the SPI
online catalog. The perfluorinated polyphenyl ether diffusion pump
fluids Fomblin Y-25/9 and Krytox 1625 are also very good lubricants,
particularly for O-rings on rotating shafts.
--
Wilbur C. Bigelow, Professor Emeritus
Materials Sci. & Engr., Univ. of Michigan
Ann Arbor, Michigan 48109-2136
e-mail: bigelow-at-umich.edu;
Fx:734-763-4788; Ph:734-975-0858
Address mail to: 2911 Whittier Court
Ann Arbor, MI 48104-6731

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From: bigelow-at-umich.edu
Date: Tue, 12 Feb 2008 14:40:04 -0600
Subject: [Microscopy] RE: Ion pump life

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

Basically, the lifetime of ion getter pumps is determined by the
amount of titanium available in their cathodes for producing the
gettering action that is the basis of the pumps' operation, and also
by the pressure range at which the pumps are operated. This matter
is discussed in some detail in Sect. 7.1.8 (p 294) of my book Vacuum
Methods in Electron Microscopy. As noted there, most manufacturers
rate pump life on the basis of continuous operation at a pressure of
10^-6 Torr. Typical values are 45,000 to 50,000 hours (5 to 6
years). However, if the pump operates at a pressure of 10^-7 Torr
(not unusual for pumps on the electron guns of modern instruments)
then the operating life would be ten times as long, or of the order
of 50 years. The development of "flakes", whiskers, and
contamination on the insulators can shorten pump life, as mentioned
by others. All of these factors are discussed in the above reference..
--
Wilbur C. Bigelow, Professor Emeritus
Materials Sci. & Engr., Univ. of Michigan
Ann Arbor, Michigan 48109-2136
e-mail: bigelow-at-umich.edu;
Fx:734-763-4788; Ph:734-975-0858
Address mail to: 2911 Whittier Court
Ann Arbor, MI 48104-6731

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From: wesley-smith-at-ukzn.ac.za
Date: Tue, 12 Feb 2008 17:49:27 -0600
Subject: [Microscopy] viaWWW: Polaron E6300 vacuum evaporator circuit diagram

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Email: wesley-smith-at-ukzn.ac.za
Name: James Wesley-Smith

Organization: University of KwaZulu-Natal, Durban, South Africa

Title-Subject: [Filtered] Polaron E6300 vacuum evaporator circuit diagram

Question: Dear colleagues
If anyone out there has a Polaron E6300 vacuum evaporator, I would
really appreciate if you could send me a scanned
copy of the circuit diagramn needed for some troubleshooting.

Many thanks in advance!

James


Dr James Wesley-Smith
Electron Microscope Unit
University of KZN, Westville Campus
Private Bag X54001
Durban 4000
South Africa

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From: z.zhou-at-sheffield.ac.uk
Date: Tue, 12 Feb 2008 17:49:53 -0600
Subject: [Microscopy] viaWWW: carbon contamination while doing EELS

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Email: z.zhou-at-sheffield.ac.uk
Name: Zoe

Title-Subject: [Filtered] carbon contamination while doing EELS

Question: I found bad carbon contamination while put Cr3C2 samples in
a 2010 FEGTEM for EELS analysis. They were thin film cross sections
made by conventional sandwich method by Epoxy glue, and Gatan PIPS
ion milling. I have examined three samples made by the same route,
two turned out contaminated easily, but one seemed not much affected.
The samples were subjected to selected area EELS in diffraction mode
and STEM ADF imaiging. Carbon accumulated at the edge of the selected
area circle. Once the beam was focused, carbon K-edge was enchanced
in the EELS acquired. Amorphous carbon in EEL spectra stops me from
studying the real carbon bonding from the Cr3C2 phase.

My questions are:
(1)Why were some samples contaminated, other not much?
(2)What could be the most possible contamination sources?
(3)How can I minimise the contamination both during sample
preperation and TEM examination?
(3)How reliable is the carbon data acquired?

Zoe

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From: walck-at-southbaytech.com
Date: Tue, 12 Feb 2008 19:46:28 -0600
Subject: [Microscopy] viaWWW: carbon contamination while doing EELS

Contents Retrieved from Microscopy Listserver Archives
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Let me hazard a guess or two.

I suspect that may be breaking down your carbide to form your amorphous
carbon when you are focusing the beam onto the sample.

I had a sample of a pulsed laser deposited diamond-like carbon film. You
can see an image of this film on our website in the application note #59
(http://www.southbaytech.com/appnotes/59%20EELS%20of%20PLD%20DLC.pdf) that
was prepared by MicroCleaving(TM). The film was amorphous, but there are
alternating light and dark bands in the DLC film. EELS showed that the
darker bands were SP3 bonding while the light bands were SP2/SP3 or more
graphitic. We only had a parallel EELS on a CM200FEG. When the spot was
focused down in order to isolate a dark band, the earliest EELS spectra
showed no Pi-star peak, but almost instantly, started growing one and a spot
formed. If the beam was spread out, no contamination was seen. It was only
in the highly focused beam that we got it and in the first instant, you
could clearly see that the dark bands had no SP2 bonding. I always wanted
to revisit these samples with a GIF to examine the sample without the
conversion, similar to what Jim Bentley did with his GIF and carbon films.

Another question for you if you think that it is actual contamination is
have you plasma cleaned your sample? If you always plasma clean your samples
before putting them in the microscope and other samples do not contaminate
in your microscope, then the source is not your sample and not your
microscope, but is probably the mechanism that I described above.

For a source of contamination, check the O-rings and lubrication on your
whisper lock on the PIPS. The same Ar gas that is used for the guns is used
for the lift assembly. A colleague of mine has demonstrated conclusively
that the Ar gas was contaminated by the lubrication from the lift mechanism
in the PIPS. We strongly advise our customers who have either a Gentle
Mill(TM) or an IV3/4 equipped with a low energy gun to not share the gas
line with a PIPS instrument for that reason. Your difference in
contamination could be the amount of time the samples were left in the PIPS.
However, if you plasma clean your samples, you will eliminate this source or
any other external source of contamination on your samples.


Disclaimer: South Bay Technology manufactures and sells the MicroCleave(TM)
Kit and the PC-2000 Plasma Cleaner. We also distribute the Technoorg-Linda
Gentle Mill(TM) and IV3/4 ion mills in the United States.


-Scott

Scott D. Walck, Ph.D.
Technical Director
South Bay Technology, Inc.
1120 Via Callejon
San Clemente, CA 92673

US Toll Free: 1-800-728-2233
Tel: (949) 492-2600
Fax: (949) 492-1499

www.southbaytech.com
walck-at-southbaytech.com

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Email: z.zhou-at-sheffield.ac.uk
Name: Zoe

Title-Subject: [Filtered] carbon contamination while doing EELS

Question: I found bad carbon contamination while put Cr3C2 samples in a 2010
FEGTEM for EELS analysis. They were thin film cross sections made by
conventional sandwich method by Epoxy glue, and Gatan PIPS ion milling. I
have examined three samples made by the same route, two turned out
contaminated easily, but one seemed not much affected.
The samples were subjected to selected area EELS in diffraction mode and
STEM ADF imaiging. Carbon accumulated at the edge of the selected area
circle. Once the beam was focused, carbon K-edge was enchanced in the EELS
acquired. Amorphous carbon in EEL spectra stops me from studying the real
carbon bonding from the Cr3C2 phase.

My questions are:
(1)Why were some samples contaminated, other not much?
(2)What could be the most possible contamination sources?
(3)How can I minimise the contamination both during sample preperation and
TEM examination?
(3)How reliable is the carbon data acquired?

Zoe

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From: RCsencsits-at-lbl.gov
Date: Tue, 12 Feb 2008 23:25:04 -0600
Subject: [Microscopy] Re: viaWWW: carbon contamination while doing EELS

Contents Retrieved from Microscopy Listserver Archives
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Dear Zoe,

I have had the same experience with many different samples. The
contamination is one the sample and why or how some are cleaner than
others seems to be a mystery. However it must be correlated to
cleanliness of glues, acetone, and alcohols used during preparation.
Try to keep them clean, generally not sharing with others helps.
After a soak, follow with a rinse of fresh liquid before drying with
clean air.

If possible plasma clean your specimens before putting them in the
scope. Any plasma cleaning will help, but I have found the H2/O2
recipes superior to Ar or Ar/O2.

I am assuming that you are using the liquid N2 cold trap on the 2010.
Have is cold before inserting the sample.

If you have some old liquid freon in the lab, you can use it to rinse
the sample before inserting in the TEM. This is a great help, but not
for the environment.

If you do not have freon, or access to a plasma cleaner, and must work
with the samples as they are, then you could try "locking the carbon
in place on the surface of the sample". This might be done by using a
large spot size beam spread over a relatively large area, to bake the
carbon in place. I am not sure how well this works or for how long
you have to let the beam set to be useful, but others will probably
offer advice on this approach.

Good luck. You are not alone in your plight.

Roseann


Roseann Csencsits, PhD
Donner TEM Facility Manager
Lawrence Berkeley Lab 01-365
1 Cyclotron Road
Berkeley, CA 94720
510-486-4548





On Feb 12, 2008, at 4:01 PM, z.zhou-at-sheffield.ac.uk wrote:

}
}
} Email: z.zhou-at-sheffield.ac.uk
} Name: Zoe
}
} Title-Subject: [Filtered] carbon contamination while doing EELS
}
} Question: I found bad carbon contamination while put Cr3C2 samples in
} a 2010 FEGTEM for EELS analysis. They were thin film cross sections
} made by conventional sandwich method by Epoxy glue, and Gatan PIPS
} ion milling. I have examined three samples made by the same route,
} two turned out contaminated easily, but one seemed not much affected.
} The samples were subjected to selected area EELS in diffraction mode
} and STEM ADF imaiging. Carbon accumulated at the edge of the selected
} area circle. Once the beam was focused, carbon K-edge was enchanced
} in the EELS acquired. Amorphous carbon in EEL spectra stops me from
} studying the real carbon bonding from the Cr3C2 phase.
}
} My questions are:
} (1)Why were some samples contaminated, other not much?
} (2)What could be the most possible contamination sources?
} (3)How can I minimise the contamination both during sample
} preperation and TEM examination?
} (3)How reliable is the carbon data acquired?
}
} Zoe


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From: bigelow-at-umich.edu
Date: Wed, 13 Feb 2008 14:16:12 -0600
Subject: [Microscopy] RE: perfluorinated cmpds in EMs

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html

The reason many microscopists don't want to use perfluorinated
compounds in their electron microscopes goes back to the 1970s when
diffusion pump oils based on these compounds were first introduced.
(See Sect.5..4.5 p. 186 of "Vacuum Methods in Electron Microscopy")
When first put into use as diffusion pump fluids it was found that
these compounds broke down into small molecular fragments which were
easily pumped out of the vacuum system, and were therefore
essentially non-contaminating. Eureka! It was thought that the
problem of oil contamination from diffusion pumps was solved.
HOWEVER, after some use it was found that instruments using these
fluids developed high-voltage instabilities due to micro-discharges
along the ceramic insulators in their electron guns. This problem
was more severe in TEMS, which operate at higher accelerating
voltages, than in SEMs. About that time the Santovac
polyphenyl-ether fluids came along, and most microscopists adopted
them for use in their diffusion pumps..

I have not heard of anyone having this problem from the use of the
Brayco or Krytox vacuum greases on O-rings, even on those in specimen
stage mechanisms, however, and they are superb vacuum greases.
They are excellent lubricants, they don't migrate or bleed, they are
stable at temperatures up to around 250 C, and have vapor pressures
in the 10^-10 Torr range.

I have not had any experience with the Santovac-5GB grease, but it
sounds very interesting, too.
--
Wilbur C. Bigelow, Professor Emeritus
Materials Sci. & Engr., Univ. of Michigan
Ann Arbor, Michigan 48109-2136
e-mail: bigelow-at-umich.edu;
Fx:734-763-4788; Ph:734-975-0858
Address mail to: 2911 Whittier Court
Ann Arbor, MI 48104-6731

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From: curtp-at-binghamton.edu
Date: Wed, 13 Feb 2008 16:01:00 -0600
Subject: [Microscopy] Electron Microscopy Technician position available

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Position available at Binghamton University, one of the four
university centers of the State University of New York, for an
experienced electron microscopist to manage a facility that serves
users in biological and materials sciences. Responsibilities include
instrument maintenance (Hitachi H-7000 TEM, Hitachi S-570LB SEM),
training users, service work. Applicants should have broad expertise
in techniques for specimen preparation. Experience with light
microscopic digital imaging also desirable. Bachelor's required;
Master's preferred. Salary commensurate with education and
experience. More information and application online at http://
binghamton.interviewexchange.com/. Screening of applications will
begin March 1 and will continue until position is filled. The State
University of New York and Binghamton University are Equal
Opportunity/Affirmative Action Employers.

Dr. Curt Pueschel
Associate Professor
Department of Biological Sciences
Binghamton University
Binghamton, NY 13902-6000
607-777-2602

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From: a.c.richardson-at-durham.ac.uk
Date: Wed, 13 Feb 2008 16:18:24 -0600
Subject: [Microscopy] Freeze substitution

Contents Retrieved from Microscopy Listserver Archives
http://www.microscopy.com/MicroscopyListserver/MicroscopyArchives.html


Dear List members,
I am trying to source a UK or European supplier of anhydrous glutaraldehyde in
acetone for use in freeze substitution protocols.
Does anyone know of or have a preferred supplier?
Thanks in advance.
Christine.
--

A.Christine.Richardson
Laboratory Manager
University of Durham
School of Biological & Biomedical Science
Centre for Molecular Imaging
Science site
South Rd
Durham
England
DH1 3LE
Tel: 0191 3341285\3341321
Fax: 0191 3341201
E-mail: microscopy.unit-at-dur.ac.uk

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3,