Re: [Histonet] Tissue Fixation
If the specimen is placed on absorbent paper prior to fixation, the paper will gradually absorb the water from the specimen causing it to dry out. Microscopically the tissue will look a little like what you see when a laser scalpel is used to excise a skin specimen. The heat affected eosin stained collagen will look quite brilliant (even fluorescent like) and if you do a Masson stain for connective tissue will give a red colouration, rather than a green or blue you would normally see with well-fixed collagen. Regards Tony Henwood JP, MSc, BAppSc, GradDipSysAnalys, CT(ASC), FFSc(RCPA) Principal Scientist, the Children's Hospital at Westmead Adjunct Fellow, School of Medicine, University of Western Sydney Tel: 612 9845 3306 Fax: 612 9845 3318 Pathology Department the children's hospital at westmead Cnr Hawkesbury Road and Hainsworth Street, Westmead Locked Bag 4001, Westmead NSW 2145, AUSTRALIA -Original Message- From: T H via Histonet [mailto:histonet@lists.utsouthwestern.edu] Sent: Friday, 31 March 2017 11:51 PM To: histonet@lists.utsouthwestern.edu Subject: [Histonet] Tissue Fixation Good Morning, I have a pathologist that is not happy with the fixation on some of our LEEP specimens. She swears its histology doing something to the specimen to cause the tissue to look unfixed on only "part" of the LEEP specimens (all the same client specimens). She claims we must be diluting our formalin to cause this issue or "something". We mentioned maybe it was on the clients end not placing them in 10% formalin right away, she wouldn't hear of it. Let me give you some back ground on how our process works. Our clients send us all our specimens to us via Overnight FedEx or UPS in 10% formalin they will then they sit in 10% formalin in-house until the processors are started around 3pm and sits an additional 5 hours in 10% formalin on the processor before the processor actually starts. That being said the fixation process has had a pretty good start before we ever even touch it. My question is, and I thought I had read this in the past is, when a specimen is left out prior to fixation and lying on a absorbent surface such as a paper towel, won't the area of the tissue touching the absorbent surface begin the disintegration processes faster in that exact area then the rest of the specimen? Or if you have any other suggestion on what might be happening to only "certain" specimens would be great as well. Thanks for your help! Tim ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet This message is intended for the addressee named and may contain confidential information. If you are not the intended recipient, please delete it and notify the sender. Views expressed in this message are those of the individual sender, and are not necessarily the views of NSW Health or any of its entities. ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
Re: [Histonet] Tissue fixation
Tim describes a problem "I have a pathologist that is not happy with the fixation on some of our LEEP specimens." LEEP specimens are inherently crappy, because of the cautery used to obtain them, and the resulting cautery artifact in the specimens. In the last few years they've turned the voltage down, and that's helped some - and perhaps this particular clinic hasn't turned the voltage down. I wonder how familiar your pathologist is with the whole process - the sort of homely detail not taught in pathology residency, and the sort of detail I often go out and research on my own. It's helpful to all to know that the clinical stakes here are not high - we do report margins on cervical LEEP specimens (when we can figure them out), but clinical outcomes apparently don't have much to do with whether margins are positive for dysplasia or not. It's impossible to get india ink to stick to the cauterized gross margins, but the cautery artifact is painfully obvious under the microscope anyway. Bob Richmond Samurai Pathologist Maryville TN ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
Re: [Histonet] Tissue fixation
I agree with Rene. To discredit the pathologist theory show if all of the specimens from the run are not fixed properly. Then show if it is just the LEEPs. Then show if it is that particular clients specimens? Then onto that client's LEEPs. That should prove your problem lies with the client handling and not the fixation on your end. Cauterization can cause burning of the specimen, but not look unfixed. If it was left out of formalin, autolysis can set in. The situation shows the god-complex some physicians have and the lack of respect they have for their techs. This is why we should all be certified and keep up with continuing education, so that these pathologists will respect us. Ok, I'm going to get off my soapbox now, before I say something ugly. Toysha Mayer -- Message: 3 Date: Fri, 31 Mar 2017 12:50:37 + From: T H <thiggin...@msn.com> To: "histonet@lists.utsouthwestern.edu" <histonet@lists.utsouthwestern.edu> Subject: [Histonet] Tissue Fixation Message-ID: <sn1pr19mb060735d7b896c67b0223e098d8...@sn1pr19mb0607.namprd19.prod.outlook.com> Content-Type: text/plain; charset="iso-8859-1" Good Morning, I have a pathologist that is not happy with the fixation on some of our LEEP specimens. She swears its histology doing something to the specimen to cause the tissue to look unfixed on only "part" of the LEEP specimens (all the same client specimens). She claims we must be diluting our formalin to cause this issue or "something". We mentioned maybe it was on the clients end not placing them in 10% formalin right away, she wouldn't hear of it. Let me give you some back ground on how our process works. Our clients send us all our specimens to us via Overnight FedEx or UPS in 10% formalin they will then they sit in 10% formalin in-house until the processors are started around 3pm and sits an additional 5 hours in 10% formalin on the processor before the processor actually starts. That being said the fixation process has had a pretty good start before we ever even touch it. My question is, and I thought I had read this in the past is, when a specimen is left out prior to fixation and lying on a absorbent surface such as a paper towel, won't the area of the tissue touching the absorbent surface begin the disintegration processes faster in that exact area then the rest of the specimen? Or if you have any other suggestion on what might be happening to only "certain" specimens would be great as well. Thanks for your help! Tim -- Message: 4 Date: Fri, 31 Mar 2017 13:32:35 + (UTC) From: Rene J Buesa <rjbu...@yahoo.com> To: T H <thiggin...@msn.com>, "histonet@lists.utsouthwestern.edu" <histonet@lists.utsouthwestern.edu> Subject: Re: [Histonet] Tissue Fixation Message-ID: <1730848134.8065268.1490967155...@mail.yahoo.com> Content-Type: text/plain; charset=UTF-8 What you describe as a possible scenario is absolutely possible.If your PT does not "want to hear" about it, suggest she gets a "hearing aid" or to study something about histotechnology or even better yet, pay attention to what a professional on the subject (you) has to say about it. You would never dare to question her diagnosis, why would she question yours on this subject?Ren? On Friday, March 31, 2017 9:11 AM, T H via Histonet <histonet@lists.utsouthwestern.edu> wrote: Good Morning, I have a pathologist that is not happy with the fixation on some of our LEEP specimens.? She swears its histology doing something to the specimen to cause the tissue to look unfixed on only "part" of the LEEP specimens (all the same client specimens).? She claims we must be diluting our formalin to cause this issue or "something".? We mentioned maybe it was on the clients end not placing them in 10% formalin right away, she wouldn't hear of it. Let me give you some back ground on how our process works.? Our clients send us all our specimens to us via Overnight FedEx or UPS in 10% formalin they will then they sit in 10% formalin in-house until the processors are started around 3pm and sits an additional 5 hours in 10% formalin on the processor before the processor actually starts.? That being said the fixation process has had a pretty good start before we ever even touch it. My question is, and I thought I had read this in the past is, when a specimen is left out prior to fixation and lying on a absorbent surface such as a paper towel, won't the area of the tissue touching the absorbent surface begin the disintegration processes faster in that exact area then the rest of the specimen?? Or if you have any other suggestion on what might be happening to only "certain" specimens would be great as well. Thanks for your help! Tim ___
Re: [Histonet] Tissue Fixation
I second the opinion of Joyce. We see such effects in portio-conisations, that are done with a thermo-electrical knife. The surface and the underlying area show a very pink colour in HE. It can also be seen in prostata-chips. IHC on such biopsies shows the effect of an non-stainable edge with a clear cut between positive and negative. https://www.uni-marburg.de/fb20/zahnerhaltk/lehre/Download/Bilder/35_plattenepithelmetaplasie_portio_02212427.jpg I've found this picture, that shows a typical conisation-section. regards Gudrun -Ursprüngliche Nachricht- Von: Weems, Joyce K. via Histonet [mailto:histonet@lists.utsouthwestern.edu] Gesendet: Freitag, 31. März 2017 17:26 An: Morken, Timothy; Rene J Buesa; T H; Histonet@lists.utsouthwestern.edu Betreff: Re: [Histonet] Tissue Fixation Aren't LEEPS done with some sort of electric method that will damage the tissue before it even reaches formalin. I'm not positive but Google it - I believe that might be the problem. j Joyce Weems Pathology Manager 678-843-7376 Phone 678-843-7831 Fax 770-380-8099 Cell joyce.we...@emoryhealthcare.org www.saintjosephsatlanta.org 5665 Peachtree Dunwoody Road Atlanta, GA 30342 This e-mail, including any attachments is the property of Saint Joseph’s Hospital and is intended for the sole use of the intended recipient(s). It may contain information that is privileged and confidential. Any unauthorized review, use, disclosure, or distribution is prohibited. If you are not the intended recipient, please delete this message, and reply to the sender regarding the error in a separate email. -Original Message- From: Morken, Timothy via Histonet [mailto:histonet@lists.utsouthwestern.edu] Sent: Friday, March 31, 2017 11:07 AM To: Rene J Buesa <rjbu...@yahoo.com>; T H <thiggin...@msn.com> Cc: Histonet <histonet@lists.utsouthwestern.edu> Subject: Re: [Histonet] Tissue Fixation Tim, I have to agree with Rene that the formalin or time in formalin is obviously not the problem - it has plenty of time in formalin (and who would dilute it anyway?). Handling before formalin must always be determined when problems arise. If the sample sits on a paper towel, gauze etc it does not really degrade faster, rather the tissue may dry out and so fixes by dehydration rather than by formalin. It may be the formalin cannot get into the tissue in those dried out portions of the tissue. However that is just speculation. Since these all seem to be from one particular client, the client is the place to start. The only way to determine the problem is to follow the specimen from start to finish. Can you or someone you trust physically observe the way samples are handled from the time they are taken to the time put in formalin? One issue I always run up against is people saying they do one thing but actually doing another. And they may realize during questioning that they are not doing it right but don't want to admit it. It wastes a lot of time. I've had physicians tell me to ignore the part of the process they are responsible for because they do it right. I just tell them that to be complete we need to follow the process from start to finish, nothing personal, just business. Leaving any part out may lead to not resolving the problem. Probably 99% of the process is just fine, but that 1% is damaging the sample and needs to be illuminated. Tim Morken Pathology Site Manager, Parnassus Supervisor, Electron Microscopy/Neuromuscular Special Studies Department of Pathology UC San Francisco Medical Center -Original Message- From: Rene J Buesa via Histonet [mailto:histonet@lists.utsouthwestern.edu] Sent: Friday, March 31, 2017 6:33 AM To: T H; histonet@lists.utsouthwestern.edu Subject: Re: [Histonet] Tissue Fixation What you describe as a possible scenario is absolutely possible.If your PT does not "want to hear" about it, suggest she gets a "hearing aid" or to study something about histotechnology or even better yet, pay attention to what a professional on the subject (you) has to say about it. You would never dare to question her diagnosis, why would she question yours on this subject?René On Friday, March 31, 2017 9:11 AM, T H via Histonet <histonet@lists.utsouthwestern.edu> wrote: Good Morning, I have a pathologist that is not happy with the fixation on some of our LEEP specimens. She swears its histology doing something to the specimen to cause the tissue to look unfixed on only "part" of the LEEP specimens (all the same client specimens). She claims we must be diluting our formalin to cause this issue or "something". We mentioned maybe it was on the clients end not placing them in 10% formalin right away, she wouldn't hear of it. Let me give you some back ground on how our process works. Our clients send us all our specimens to us via Overnight FedEx or UPS in 10% formalin they will then they sit in 10% formali
Re: [Histonet] Tissue Fixation
Aren't LEEPS done with some sort of electric method that will damage the tissue before it even reaches formalin. I'm not positive but Google it - I believe that might be the problem. j Joyce Weems Pathology Manager 678-843-7376 Phone 678-843-7831 Fax 770-380-8099 Cell joyce.we...@emoryhealthcare.org www.saintjosephsatlanta.org 5665 Peachtree Dunwoody Road Atlanta, GA 30342 This e-mail, including any attachments is the property of Saint Joseph’s Hospital and is intended for the sole use of the intended recipient(s). It may contain information that is privileged and confidential. Any unauthorized review, use, disclosure, or distribution is prohibited. If you are not the intended recipient, please delete this message, and reply to the sender regarding the error in a separate email. -Original Message- From: Morken, Timothy via Histonet [mailto:histonet@lists.utsouthwestern.edu] Sent: Friday, March 31, 2017 11:07 AM To: Rene J Buesa <rjbu...@yahoo.com>; T H <thiggin...@msn.com> Cc: Histonet <histonet@lists.utsouthwestern.edu> Subject: Re: [Histonet] Tissue Fixation Tim, I have to agree with Rene that the formalin or time in formalin is obviously not the problem - it has plenty of time in formalin (and who would dilute it anyway?). Handling before formalin must always be determined when problems arise. If the sample sits on a paper towel, gauze etc it does not really degrade faster, rather the tissue may dry out and so fixes by dehydration rather than by formalin. It may be the formalin cannot get into the tissue in those dried out portions of the tissue. However that is just speculation. Since these all seem to be from one particular client, the client is the place to start. The only way to determine the problem is to follow the specimen from start to finish. Can you or someone you trust physically observe the way samples are handled from the time they are taken to the time put in formalin? One issue I always run up against is people saying they do one thing but actually doing another. And they may realize during questioning that they are not doing it right but don't want to admit it. It wastes a lot of time. I've had physicians tell me to ignore the part of the process they are responsible for because they do it right. I just tell them that to be complete we need to follow the process from start to finish, nothing personal, just business. Leaving any part out may lead to not resolving the problem. Probably 99% of the process is just fine, but that 1% is damaging the sample and needs to be illuminated. Tim Morken Pathology Site Manager, Parnassus Supervisor, Electron Microscopy/Neuromuscular Special Studies Department of Pathology UC San Francisco Medical Center -Original Message- From: Rene J Buesa via Histonet [mailto:histonet@lists.utsouthwestern.edu] Sent: Friday, March 31, 2017 6:33 AM To: T H; histonet@lists.utsouthwestern.edu Subject: Re: [Histonet] Tissue Fixation What you describe as a possible scenario is absolutely possible.If your PT does not "want to hear" about it, suggest she gets a "hearing aid" or to study something about histotechnology or even better yet, pay attention to what a professional on the subject (you) has to say about it. You would never dare to question her diagnosis, why would she question yours on this subject?René On Friday, March 31, 2017 9:11 AM, T H via Histonet <histonet@lists.utsouthwestern.edu> wrote: Good Morning, I have a pathologist that is not happy with the fixation on some of our LEEP specimens. She swears its histology doing something to the specimen to cause the tissue to look unfixed on only "part" of the LEEP specimens (all the same client specimens). She claims we must be diluting our formalin to cause this issue or "something". We mentioned maybe it was on the clients end not placing them in 10% formalin right away, she wouldn't hear of it. Let me give you some back ground on how our process works. Our clients send us all our specimens to us via Overnight FedEx or UPS in 10% formalin they will then they sit in 10% formalin in-house until the processors are started around 3pm and sits an additional 5 hours in 10% formalin on the processor before the processor actually starts. That being said the fixation process has had a pretty good start before we ever even touch it. My question is, and I thought I had read this in the past is, when a specimen is left out prior to fixation and lying on a absorbent surface such as a paper towel, won't the area of the tissue touching the absorbent surface begin the disintegration processes faster in that exact area then the rest of the specimen? Or if you have any other suggestion on what might be happening to only "certain" specimens would be great as well. Thanks for your help! Tim ___ Histonet mailing list
Re: [Histonet] Tissue Fixation
Tim, I have to agree with Rene that the formalin or time in formalin is obviously not the problem - it has plenty of time in formalin (and who would dilute it anyway?). Handling before formalin must always be determined when problems arise. If the sample sits on a paper towel, gauze etc it does not really degrade faster, rather the tissue may dry out and so fixes by dehydration rather than by formalin. It may be the formalin cannot get into the tissue in those dried out portions of the tissue. However that is just speculation. Since these all seem to be from one particular client, the client is the place to start. The only way to determine the problem is to follow the specimen from start to finish. Can you or someone you trust physically observe the way samples are handled from the time they are taken to the time put in formalin? One issue I always run up against is people saying they do one thing but actually doing another. And they may realize during questioning that they are not doing it right but don't want to admit it. It wastes a lot of time. I've had physicians tell me to ignore the part of the process they are responsible for because they do it right. I just tell them that to be complete we need to follow the process from start to finish, nothing personal, just business. Leaving any part out may lead to not resolving the problem. Probably 99% of the process is just fine, but that 1% is damaging the sample and needs to be illuminated. Tim Morken Pathology Site Manager, Parnassus Supervisor, Electron Microscopy/Neuromuscular Special Studies Department of Pathology UC San Francisco Medical Center -Original Message- From: Rene J Buesa via Histonet [mailto:histonet@lists.utsouthwestern.edu] Sent: Friday, March 31, 2017 6:33 AM To: T H; histonet@lists.utsouthwestern.edu Subject: Re: [Histonet] Tissue Fixation What you describe as a possible scenario is absolutely possible.If your PT does not "want to hear" about it, suggest she gets a "hearing aid" or to study something about histotechnology or even better yet, pay attention to what a professional on the subject (you) has to say about it. You would never dare to question her diagnosis, why would she question yours on this subject?René On Friday, March 31, 2017 9:11 AM, T H via Histonet <histonet@lists.utsouthwestern.edu> wrote: Good Morning, I have a pathologist that is not happy with the fixation on some of our LEEP specimens. She swears its histology doing something to the specimen to cause the tissue to look unfixed on only "part" of the LEEP specimens (all the same client specimens). She claims we must be diluting our formalin to cause this issue or "something". We mentioned maybe it was on the clients end not placing them in 10% formalin right away, she wouldn't hear of it. Let me give you some back ground on how our process works. Our clients send us all our specimens to us via Overnight FedEx or UPS in 10% formalin they will then they sit in 10% formalin in-house until the processors are started around 3pm and sits an additional 5 hours in 10% formalin on the processor before the processor actually starts. That being said the fixation process has had a pretty good start before we ever even touch it. My question is, and I thought I had read this in the past is, when a specimen is left out prior to fixation and lying on a absorbent surface such as a paper towel, won't the area of the tissue touching the absorbent surface begin the disintegration processes faster in that exact area then the rest of the specimen? Or if you have any other suggestion on what might be happening to only "certain" specimens would be great as well. Thanks for your help! Tim ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
Re: [Histonet] Tissue Fixation
Bravo Rene! Paula Keene Pierce, BS, HTL(ASCP)HTPresidentExcalibur Pathology, Inc.5830 N Blue Lake DriveNorman, OK 73069PH 405-759-3953FAX 405-759-7513www.excaliburpathology.com From: Rene J Buesa via Histonet <histonet@lists.utsouthwestern.edu> To: T H <thiggin...@msn.com>; "histonet@lists.utsouthwestern.edu" <histonet@lists.utsouthwestern.edu> Sent: Friday, March 31, 2017 8:44 AM Subject: Re: [Histonet] Tissue Fixation What you describe as a possible scenario is absolutely possible.If your PT does not "want to hear" about it, suggest she gets a "hearing aid" or to study something about histotechnology or even better yet, pay attention to what a professional on the subject (you) has to say about it. You would never dare to question her diagnosis, why would she question yours on this subject?René On Friday, March 31, 2017 9:11 AM, T H via Histonet <histonet@lists.utsouthwestern.edu> wrote: Good Morning, I have a pathologist that is not happy with the fixation on some of our LEEP specimens. She swears its histology doing something to the specimen to cause the tissue to look unfixed on only "part" of the LEEP specimens (all the same client specimens). She claims we must be diluting our formalin to cause this issue or "something". We mentioned maybe it was on the clients end not placing them in 10% formalin right away, she wouldn't hear of it. Let me give you some back ground on how our process works. Our clients send us all our specimens to us via Overnight FedEx or UPS in 10% formalin they will then they sit in 10% formalin in-house until the processors are started around 3pm and sits an additional 5 hours in 10% formalin on the processor before the processor actually starts. That being said the fixation process has had a pretty good start before we ever even touch it. My question is, and I thought I had read this in the past is, when a specimen is left out prior to fixation and lying on a absorbent surface such as a paper towel, won't the area of the tissue touching the absorbent surface begin the disintegration processes faster in that exact area then the rest of the specimen? Or if you have any other suggestion on what might be happening to only "certain" specimens would be great as well. Thanks for your help! Tim ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
Re: [Histonet] Tissue Fixation
What you describe as a possible scenario is absolutely possible.If your PT does not "want to hear" about it, suggest she gets a "hearing aid" or to study something about histotechnology or even better yet, pay attention to what a professional on the subject (you) has to say about it. You would never dare to question her diagnosis, why would she question yours on this subject?René On Friday, March 31, 2017 9:11 AM, T H via Histonetwrote: Good Morning, I have a pathologist that is not happy with the fixation on some of our LEEP specimens. She swears its histology doing something to the specimen to cause the tissue to look unfixed on only "part" of the LEEP specimens (all the same client specimens). She claims we must be diluting our formalin to cause this issue or "something". We mentioned maybe it was on the clients end not placing them in 10% formalin right away, she wouldn't hear of it. Let me give you some back ground on how our process works. Our clients send us all our specimens to us via Overnight FedEx or UPS in 10% formalin they will then they sit in 10% formalin in-house until the processors are started around 3pm and sits an additional 5 hours in 10% formalin on the processor before the processor actually starts. That being said the fixation process has had a pretty good start before we ever even touch it. My question is, and I thought I had read this in the past is, when a specimen is left out prior to fixation and lying on a absorbent surface such as a paper towel, won't the area of the tissue touching the absorbent surface begin the disintegration processes faster in that exact area then the rest of the specimen? Or if you have any other suggestion on what might be happening to only "certain" specimens would be great as well. Thanks for your help! Tim ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
[Histonet] Tissue Fixation
Good Morning, I have a pathologist that is not happy with the fixation on some of our LEEP specimens. She swears its histology doing something to the specimen to cause the tissue to look unfixed on only "part" of the LEEP specimens (all the same client specimens). She claims we must be diluting our formalin to cause this issue or "something". We mentioned maybe it was on the clients end not placing them in 10% formalin right away, she wouldn't hear of it. Let me give you some back ground on how our process works. Our clients send us all our specimens to us via Overnight FedEx or UPS in 10% formalin they will then they sit in 10% formalin in-house until the processors are started around 3pm and sits an additional 5 hours in 10% formalin on the processor before the processor actually starts. That being said the fixation process has had a pretty good start before we ever even touch it. My question is, and I thought I had read this in the past is, when a specimen is left out prior to fixation and lying on a absorbent surface such as a paper towel, won't the area of the tissue touching the absorbent surface begin the disintegration processes faster in that exact area then the rest of the specimen? Or if you have any other suggestion on what might be happening to only "certain" specimens would be great as well. Thanks for your help! Tim ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
Re: [Histonet] tissue fixation-formaldehyde concentrations which is best.
There are many books on histological technique. Most of them are expensive. The 5th edition of John Kiernan's excellent HISTOLOGICAL AND HISTOCHEMICAL METHODS will sell for $100 when it comes out in July. If that is too much for your budget, there are older books that cover 95% of what you need to know. The 4th edition of Kiernan's HISTOLOGICAL AND HISTOCHEMICAL METHODS is available used for $60, but the price may fall when the 5th edition comes out. A used 4th edition of Gretchen Humason's ANIMAL TISSUE TECHNIQUES is a great bargain at $12. Allen A. Smith Professor of Anatomy Barry University School of Podiatric Medicine Miami Shores, Florida -Original Message- From: John Kiernan [mailto:jkier...@uwo.ca] Sent: Saturday, June 06, 2015 12:31 AM To: Peter Noyce; histonet@lists.utsouthwestern.edu Subject: Re: [Histonet] tissue fixation-formaldehyde concentrations which is best. Dear Peter, Some of the information you mention as anecdotal is wrong. Formaldehyde and paraformaldehyde are well documented in original peer-reviewed papers and in all textbooks in the fields of histotechnology and histochemistry. Your anecdote about high concentrations of formaldehyde quickly form a 'shell' in the tissue and will stop good penetration and fixation to the deeper tissues has no basis in published work. Paraformaldehyde is an insoluble polymer, not non polymerized formaldehyde. There is no such thing as 4% paraformaldehyde! It is a sad fact that many labs do not contain even one book about histotechnology. Nearly all books in the field (and there are many) have plenty of references to review articles and original literature about the techniques. There are also several websites that provide links to useful papers. Check out some of the useful links on the Biological Stain Commission's site: http://biologicalstaincommission.org/useful-links/ As a graduate student, you need to work from primary sources or reliable secondary sources. When you defend your thesis, you won't want to justify your fixation or staining method by saying I got the method by asking on an internet listserver. John Kiernan Professor Emeritus Anatomy Cell Biology University of Western Ontario London,Canada = = = On 05/06/15, Peter Noyce pwno...@gmail.com wrote: Formaldehyde 37% (commonly called 100% formalin) compared to 4% ( commonly known as 10% neutral buffered formalin)-in theory the 37% should fix quicker and better BUT anecdotally it is said that high concentrations of formaldehyde quickly form a shell in the tissue and will stop good penetration and fixation to the deeper tissues AND over the years it has been said anecdotally that 4% concentration is the quickest and most complete for all sample (mammal and plant) fixation and preservation-are these true. Please do discuss the methanol or buffers that is in the formaldehyde, or discuss paraformaldehyde (which is non polymerized formaldehyde with no methanol, in water). Regards Peter Noyce PhD student. ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
Re: [Histonet] tissue fixation-formaldehyde concentrations which is best.
John, I totally agree Tony From: John Kiernan [jkier...@uwo.ca] Sent: Saturday, 6 June 2015 2:31 PM To: Peter Noyce; histonet@lists.utsouthwestern.edu Subject: Re: [Histonet] tissue fixation-formaldehyde concentrations which is best. Dear Peter, Some of the information you mention as anecdotal is wrong. Formaldehyde and paraformaldehyde are well documented in original peer-reviewed papers and in all textbooks in the fields of histotechnology and histochemistry. Your anecdote about high concentrations of formaldehyde quickly form a 'shell' in the tissue and will stop good penetration and fixation to the deeper tissues has no basis in published work. Paraformaldehyde is an insoluble polymer, not non polymerized formaldehyde. There is no such thing as 4% paraformaldehyde! It is a sad fact that many labs do not contain even one book about histotechnology. Nearly all books in the field (and there are many) have plenty of references to review articles and original literature about the techniques. There are also several websites that provide links to useful papers. Check out some of the useful links on the Biological Stain Commission's site: http://biologicalstaincommission.org/useful-links/ As a graduate student, you need to work from primary sources or reliable secondary sources. When you defend your thesis, you won't want to justify your fixation or staining method by saying I got the method by asking on an internet listserver. John Kiernan Professor Emeritus Anatomy Cell Biology University of Western Ontario London,Canada = = = On 05/06/15, Peter Noyce pwno...@gmail.com wrote: Formaldehyde 37% (commonly called 100% formalin) compared to 4% ( commonly known as 10% neutral buffered formalin)-in theory the 37% should fix quicker and better BUT anecdotally it is said that high concentrations of formaldehyde quickly form a shell in the tissue and will stop good penetration and fixation to the deeper tissues AND over the years it has been said anecdotally that 4% concentration is the quickest and most complete for all sample (mammal and plant) fixation and preservation-are these true. Please do discuss the methanol or buffers that is in the formaldehyde, or discuss paraformaldehyde (which is non polymerized formaldehyde with no methanol, in water). Regards Peter Noyce PhD student. ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet * This email and any files transmitted with it are confidential and intended solely for the use of the individual or entity to whom they are addressed. If you are not the intended recipient, please delete it and notify the sender. Views expressed in this message and any attachments are those of the individual sender, and are not necessarily the views of The Sydney Children's Hospitals Network. This note also confirms that this email message has been virus scanned and although no computer viruses were detected, The Sydney Childrens Hospital's Network accepts no liability for any consequential damage resulting from email containing computer viruses. * ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
Re: [Histonet] tissue fixation-formaldehyde concentrations
I have to agree with the student, John. Sure, he is coming from ignorance ( not a bad situation: naivety is not a fault... we all are/were there at some point;-) Sure...I agree with you re the using of the word Paraformaldehyde as a fixative I often sigh when used. However, differential fixation ( zonal fixation) has always been an issue. We often see the zonal effects of this? Particularly in lymph nodes ( parenchymatous tissues) Obviously, when immersion fixing. Most often ...NOT with agitation. Respectfully, Carl Carl Hobbs FIBMS Histology and Imaging Manager Wolfson CARD Guys Campus, London Bridge Kings College London London SE1 1UL 020 7848 6813 ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
Re: [Histonet] tissue fixation-formaldehyde concentrations which is best.
Dear Peter, Some of the information you mention as anecdotal is wrong. Formaldehyde and paraformaldehyde are well documented in original peer-reviewed papers and in all textbooks in the fields of histotechnology and histochemistry. Your anecdote about high concentrations of formaldehyde quickly form a 'shell' in the tissue and will stop good penetration and fixation to the deeper tissues has no basis in published work. Paraformaldehyde is an insoluble polymer, not non polymerized formaldehyde. There is no such thing as 4% paraformaldehyde! It is a sad fact that many labs do not contain even one book about histotechnology. Nearly all books in the field (and there are many) have plenty of references to review articles and original literature about the techniques. There are also several websites that provide links to useful papers. Check out some of the useful links on the Biological Stain Commission's site: http://biologicalstaincommission.org/useful-links/ As a graduate student, you need to work from primary sources or reliable secondary sources. When you defend your thesis, you won't want to justify your fixation or staining method by saying I got the method by asking on an internet listserver. John Kiernan Professor Emeritus Anatomy Cell Biology University of Western Ontario London,Canada = = = On 05/06/15, Peter Noyce pwno...@gmail.com wrote: Formaldehyde 37% (commonly called 100% formalin) compared to 4% ( commonly known as 10% neutral buffered formalin)-in theory the 37% should fix quicker and better BUT anecdotally it is said that high concentrations of formaldehyde quickly form a shell in the tissue and will stop good penetration and fixation to the deeper tissues AND over the years it has been said anecdotally that 4% concentration is the quickest and most complete for all sample (mammal and plant) fixation and preservation-are these true. Please do discuss the methanol or buffers that is in the formaldehyde, or discuss paraformaldehyde (which is non polymerized formaldehyde with no methanol, in water). Regards Peter Noyce PhD student. ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
[Histonet] tissue fixation-formaldehyde concentrations which is best.
Formaldehyde 37% (commonly called 100% formalin) compared to 4% ( commonly known as 10% neutral buffered formalin)-in theory the 37% should fix quicker and better BUT anecdotally it is said that high concentrations of formaldehyde quickly form a shell in the tissue and will stop good penetration and fixation to the deeper tissues AND over the years it has been said anecdotally that 4% concentration is the quickest and most complete for all sample (mammal and plant) fixation and preservation-are these true. Please do discuss the methanol or buffers that is in the formaldehyde, or discuss paraformaldehyde (which is non polymerized formaldehyde with no methanol, in water). Regards Peter Noyce PhD student. ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet