RE: [Histonet] TTF-1/background staining

2011-02-03 Thread Anthony Reilly
Hi Paula
 
I do not believe that RTU Abs really exist.  No company can produce an antibody 
that is suitable for use by all laboratories taking in to consideration how 
tissue can be handled differently from lab to lab.  I have used many RTU Abs 
which I have had to dilute to get optimal staining with Cam 5.2 a good example. 
 On the Bond I was using it at 1:25.  try titreing your Ab and see if that will 
reduce/eliminate your background.
 
regards
Tony

 Debra Siena dsi...@statlab.com 4/02/2011 8:02 am 
Hi Paula,

I am probably reading between the lines here but on your TTF protocol do you 
use a streptavidin biotin detection system and if so do you block for 
endogenous biotin, liver will have endogenous biotin where lung may not have as 
much?  thanks

Debbie Siena HT(ASCP)QIHC
Technical Manager | StatLab Medical Products
Direct: 972-436-1010  x229 


-Original Message-
From: histonet-boun...@lists.utsouthwestern.edu 
[mailto:histonet-boun...@lists.utsouthwestern.edu] On Behalf Of Paula Lucas
Sent: Thursday, February 03, 2011 2:38 PM
To: histonet@lists.utsouthwestern.edu 
Subject: [Histonet] TTF-1/background staining

How can I eliminate the background or as you say, non-specific staining?



I'm no expert here, I admit, and so I'm asking for your help and
suggestions.  I have searched the Histonet archives, and a lot of what I'm
seeing deals with animal or rodent tissues, and a lot of it was confusing to
me.



To give you a little background info:

We use the Lab Vision stainer and the TTF-1 antibody we use is from Cell
Marque.  We were having issues with this marker from Lab Vision, so we
switched to TTF-1 a while ago.  We use the UltraVision LP detection kit from
Lab Vision. It's a polymer driven detection kit. 



The antibody is a ready to use, and we have the time set at 30 minutes.  



We were getting the background staining on a liver specimen last week, and
we also had this problem today on a lung case.  My doctor is getting
frustrated, and wants me to do something about this, and to repeat the TTF-1
stain on the lung, so if someone can give me some suggestions to try, I'm
ready to try them.



Thanks in advance,

Paula

Lab Manager

Bio-Path Medical Group

Fountain Valley, CA

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Re: [Histonet] lost tissue

2010-11-11 Thread Anthony Reilly
Hi Christine
 
You have had some good suggestions to date.
 
Also to consider  if you are using the Peloris racks with the individual spaces 
for cassettes I have seen this happen when cassettes are inserted into the 
racks.  As most people load cassettes with the patient details facing up, if 
not careful the lid can make contact with the cassette divider and open the 
lid.  We had this happen in my lab and now the formalin that contains the racks 
prior to processing is poured through a sieve before disposal.  We have saved 
one specimen with this process and even if it is only 1 in a million it is 
worth it.
 
As the tissue is not wrapped also consider that tissue will shrink during 
processing.
 
regards
Tony
 
 
 
 

Tony Reilly  B.App.Sc. , M.Sc.
Chief Scientist, Anatomical Pathology
Pathology Queensland-PA Laboratory
_
Clinical and Statewide Services Division| QueenslandHealth
 
Level 1, Building 15,Princess Alexandra Hospital
Ipswich Road,WOOLLOONGABBA  Qld4102
Ph: 07 3176 2412
Mob: 0402 139411
Fax: 07 3176 2930
Email: tony_rei...@health.qld.gov.au
Web:  www.health.qld.gov.au/qhcss/
 
 


 Braaten, Christine I cbraa...@cheshire-med.com 12/11/2010 1:52 am 
Hi everyone,



Has anyone had a problem with cassettes opening during processing?

Sometimes the cassettes are slightly opened at the top or bottom. We

rarely lose a specimen and it's frustrating to cause the patient to be

biopsied again with no explanation what happened to it. We use Surgipath

micro cassettes and a Peloris processor and just in the past three or

four months we have lost 2 specimens somewhere between  grossing and

embedding. The specimens are tiny skin biopsies and have no paper or

biopsy pads in the cassette with them. They are not small enough to fit

through the cassette holes.  If anyone has any ideas what might be

happening I would appreciate a response. I have been embedding for 8

years and it's just been in the recent past that this has happened.

Thanks, Christine




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[Histonet] RE: Bag Sealing system

2010-09-29 Thread Anthony Reilly
Hi Loralee
 
Try a butcher's supply store.  They sell devices they use for vacuum packing 
meat.  By removing the air from the bag the evaporation of formalin is almost 
zero and the specimens will remain intact for many years.  The bags are also 
more hardy than those sold with basic bag sealers.  This is also a cheap way of 
preserving specimens for teaching purposes though depending on the shape of the 
specimen there can be some distortion due to the vacuum process.
 
regards
Tony
 
 

Tony Reilly  B.Sc. , M.Sc.
Chief Scientist, Anatomical Pathology
Pathology Queensland-PA Laboratory
_
Clinical and Statewide Services Division| QueenslandHealth
 
Level 1, Building 15,Princess Alexandra Hospital
Ipswich Road,WOOLLOONGABBA  Qld4102
Ph: 07 3176 2412
Mob: 0402 139411
Fax: 07 3176 2930
Email: tony_rei...@health.qld.gov.au
Web:  www.health.qld.gov.au/qhcss/
 
 

 McMahon, Loralee A loralee_mcma...@urmc.rochester.edu 30/09/2010 3:47 
 am 
Milestone Medical has a really neat system.  www.milesonemed.com   It is called 
the TissueSAFE.  You will find it under preanalytical tools.  We would love to 
get one for our couriers and biospecimen repository.  We haven't purchased it 
yet.


Loralee McMahon, HTL (ASCP)
Immunohistochemistry Supervisor
Strong Memorial Hospital
Department of Surgical Pathology
(585) 275-7210

From: histonet-boun...@lists.utsouthwestern.edu 
[histonet-boun...@lists.utsouthwestern.edu] On Behalf Of Masterson_John 
[masterson_j...@allergan.com] 
Sent: Wednesday, September 29, 2010 1:26 PM
To: histonet@lists.utsouthwestern.edu 
Subject: [Histonet] Bag Sealing system

Hello,

Can anyone recommend a bag and heat sealing system for archiving/shipping  
tissue?  Thanks in advance.

John

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Re: [Histonet] HM 500 M cryostat issue

2010-09-23 Thread Anthony Reilly
Hi Andrew
 
I have not used that model cryostat so this may not be the answer but I have 
experienced this on other cryostats when the microtome has been removed for 
cleaning and decontamination and reinstalled with the handle in the incorrect 
position resulting in the counterweight being totally out of whack.  When the 
microtome is removed the handle will naturally fall to 6 o'clock however when 
it is reinstalled the handle needs to be at 12 o'clock for the balance to be 
correct.  If this is not done correctly when the handle is released the chuck 
will always return to the up position.
 
I hope this helps.
 
regards
Tony
 
 
 
 

Tony Reilly  B.Sc. , M.Sc.
Chief Scientist, Anatomical Pathology
Pathology Queensland-PA Laboratory
_
Clinical and Statewide Services Division| QueenslandHealth
 
Level 1, Building 15,Princess Alexandra Hospital
Ipswich Road,WOOLLOONGABBA  Qld4102
Ph: 07 3176 2412
Mob: 0402 139411
Fax: 07 3176 2930
Email: tony_rei...@health.qld.gov.au
Web:  www.health.qld.gov.au/qhcss/
 
 


 Andrew Burgeson nap...@siscom.net 24/09/2010 4:07 am 
Hello all,

I have recently been using an older model MICROM HM500 M
cryostat and have been experiencing an annoying problem.

When I cut a section I like to leave the top edge of the OCT
anchored by not cutting through it all the way. This way I
can pull tension on the bottom of the section with a paint
brush and flatten it out before picking it up on the slide.

The carriage that holds the chuck drifts up slightly when
I cut the section, pulling the tissue and OCT up and away
from the plate. I have never used a cryostat that had a
carriage that drifted up in that position. Over the years,
every cryostat I have used (including doing a lot of Mohs
and other interoperative work)has enabled me to stop the
handle at any position in which I need it to remain.

Anyway, this made cutting some rather challenging sections
of mouse kidney very difficult. I actually had someone stand
next to me and hold the crank in place while I took the
section (or else it would drift a bit).

My sense is that the crank mechanism has something wrong
that is causing it to not remain stationary once I take my
hand off the wheel. Recently an equipment repair service
came in and told me that the unit was designed that way and
even that if I talked to the Germans that made it, they
would say it waas designed that way. (!!) wtf?

At any rate, he took out the lead conterweight and said that
he would have to modify the handle balance to suit my
needs by cutting off some of the weight and proceeded to
get out a hack saw and started trying to saw off some lead.
He got nowhere with this and stated he would have to take
the unit into the shop to do this. He was also kind of
insulting in that he told me that what i wanted the thing to
do wasnt what it was designed to do!

Any thoughts? I have asked around a bit and other histology
techs tell me that they see the drifting as an abnormal
occurrence and that it shouldnt do it if it's working right.

I think something is off with the coupling inside or with
the calibration or balance of the wheel. Any one have a
comment? First time in 16 years I have had a repair person
tell me I am using the machine the wrong way. This repair
service is not as experienced as the one I have used for
many years and I think he knows what he is doing.

Thanks

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Re: [Histonet] decontamination of cryostat

2010-07-21 Thread Anthony Reilly
Hi Annie
 
If you look up this article or many others like it on the net the simplest and 
most effective disinfectants are 70% alcohol or one of the aldehydes for most 
organisms remembering that you are only disinfecting a hard surface with no 
visible volume of liquid containing organisms.  We are fortunate to have 2 
Thermo cryostats which have an inbuilt decontamination system using 
concentrated formaldehyde which can be run overnight performing a defrost and 
decon and as the microtome is not in the refrigerated chamber there is no 
problem with ice build up in the moving parts of the microtome.  
 
 
 American Society for Microbiology
Antiseptics and Disinfectants: Activity, Action, and Resistance
Gerald McDonnell1* and A. Denver Russell2
STERIS Corporation, St. Louis Operations, St. Louis, Missouri 63166,1 and Welsh 
School of Pharmacy, Cardiff University, Cardiff CF1 3XF, United Kingdom2
 
 
All the best
Tony
 
 
 

Tony Reilly  B.Sc. , M.Sc.
Chief Scientist, Anatomical Pathology
Pathology Queensland-PA Laboratory
_
Clinical and Statewide Services Division| QueenslandHealth
 
Level 1, Building 15,Princess Alexandra Hospital
Ipswich Road,WOOLLOONGABBA  Qld4102
Ph: 07 3176 2412
Mob: 0402 139411
Fax: 07 3176 2930
Email: tony_rei...@health.qld.gov.au
Web:  www.health.qld.gov.au/qhcss/
 
 


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RE: [Histonet] ER clone 1D5 or SP1 ?

2010-04-26 Thread Anthony Reilly
Hi
 
A large number of studies have been performed which show that 6F11 will stain a 
number of tumours that 1D5 does not and I know a number of labs who have moved 
away from 1D5 because of this.  Google 1D5 and 6F11 and you will find the 
articles.  
 
regards
Tony
 
 
 
 
 

Tony Reilly  B.Sc. , M.Sc.
Chief Scientist, Anatomical Pathology
Pathology Queensland-PA Laboratory
_
Clinical and Statewide Services Division| QueenslandHealth
 
Level 1, Building 15,Princess Alexandra Hospital
Ipswich Road,WOOLLOONGABBA  Qld4102
Ph: 07 3176 2412
Mob: 0402 139411
Fax: 07 3176 2930
Email: tony_rei...@health.qld.gov.au
Web:  www.health.qld.gov.au/qhcss/
 
 


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Re: [Histonet] Cleaning VIP Processor containers

2010-04-05 Thread Anthony Reilly
Hi Brandi
 
Do you do hot water flushes? If not the film will be a build up of the buffer 
salts from your formalin.  To flush replace your formalin containers with hot 
water and write a program to run each container for 10-15 minutes.  This will 
not only clean the retorts but the fluid lines as well.  This should be done 
weekly or at least monthly if time is an issue.
 
regards
Tony
 
 
 
 

Tony Reilly  B.Sc. , M.Sc.
Chief Scientist, Anatomical Pathology
Pathology Queensland-PA Laboratory
_
Clinical and Statewide Services Division| QueenslandHealth
 
Level 1, Building 15,Princess Alexandra Hospital
Ipswich Road,WOOLLOONGABBA  Qld4102
Ph: 07 3176 2412
Mob: 0402 139411
Fax: 07 3176 2930
Email: tony_rei...@health.qld.gov.au
Web:  www.health.qld.gov.au/qhcss/
 
 


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Re: [Histonet] Processing lavages into cell pellets...

2010-03-15 Thread Anthony Reilly
Hi Jennifer
 
I realise there are products like Histogel about of which I have no knowledge 
however I have been using agar for over 30 years because I can get it easily 
and gratis from our microbiology department.
 
My experience is to spin down the cells, remove the supernatent, then add 
fixative.  The fixation helps to protect the cells from the heat of the molten 
agar.  Heat agar until just melted to ensure minimum temperature.  After adding 
molten agar spin again in a tube to give you a button of agar with the cells 
located at the pointy end.  After the agar has set the agar button can be 
removed from the tube and stored in fixative for processing.  Although there 
may be a small number of cells in the agar,  the agar does not process well on 
a short cycle(ie 2 hours)  Process on at least a 6 hour cycle and overnight is 
OK.  When embedding, the cells if in sufficient quantity, are visible in the 
agar allowing easy orientation.
 
All the best.
 
regards
Tony
 
 
 
 

Tony Reilly
Chief Scientist, Anatomical Pathology
Pathology Queensland-PA Laboratory
_
Clinical and Statewide Services Division| QueenslandHealth
 
Level 1, Building 15,Princess Alexandra Hospital
Ipswich Road,WOOLLOONGABBA  Qld4102
Ph: 07 3176 2412
Mob: 0402 139411
Fax: 07 3176 2930
Email: tony_rei...@health.qld.gov.au
Web:  www.health.qld.gov.au/qhcss/
 
 


 Johnson, Jennifer(Hist) jennifer.john...@genzyme.com 16/03/2010 4:38 am 
 
Hi,

I am looking for a little advice from anyone who has experience
processing lavage fluid into cell pellets that can be sectioned and
stained.  I need to work out a protocol using lavages from knockout mice
that may eventually be used to look at human patients.  In both models
of disease I expect to collect a lot of macrophages.  



After reading, googling and looking up articles and the Histonet, I
have come up with the following procedure.  I would appreciate advice
or ideas from anyone who has performed any part(s) of this type of
procedure:



1.   Collect lavage in PBS (perform actual lavage on euthanized
mouse using PBS as the diluent).  Store on ice until I get back to the
lab.



Question here - because I will be collecting many samples, should I spin
them right away or keep them on ice and spin them all at once?  Should I
add a mucolytic agent (mucolexx or the like) and then store them on ice
until I get back to my lab?  I know that in mice, although it will be a
model that has lung disease, mucus will not be a problem.  However, in
the human model of the disease it may be an issue.  I need to see the
effect of the mucolytic agent on the affected cells before using it on
the patients' lavages.  

Does anyone out there use a specific mucolytic agent that they like?  I
plan on trying 2 - the Mucolexx (MSDS only lists formaldehyde) and
Richard Allan Mucolytic agent (MSDS lists formaldehyde, ethylene glycol,
methyl alcohol and polyethylene glycol).  



2.   Spin down cells at 4C for 15 minutes.  Remove supernatant.  Add
fix - either overnight or for a few hours.  



Question - if I use a mucolytic agent that contains fixative -
formaldehyde - do I have to rinse it out (resuspend the cells in PBS or
other buffer and spin again) or can I just remove the sup and add a gel
(step 4)?  Is the mucolytic agent enough of a fixative (the
Thermo/Richard Allan and Mucolexx mucolytic agents contain 0.3 or 3 %
formaldehyde)?



3.   Once the cells are pelleted, should I fix them again or just
resuspend them in a gel (something like Histogel or an agar(ose)?  Does
anyone out there use either of these gels to look at cells?  Any
preferences?  



4.   Once the cells are in the gel, fix the cell pellet.  (Is this
necessary?)



5.   Pray and process the pellet into paraffin (and maybe plastic
too).



Thanks in advance for any help you can give.  



Jenn



Jennifer Johnson

Genzyme Corp.

Department of Pathology

5 Mountain Road

Framingham, MA 01701-9322

Phn - 508-271-3610

Fax - 508-872-9080



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Re: [Histonet] tb-controls selfmade

2010-03-15 Thread Anthony Reilly
Hi Gudren
 
I have not done this with TB but I have with other bacteria to produce controls 
for gram stains.  You need to have the tissue in a nutrient broth appropriate 
for the organism.  You need to consult with a laboratory that specialises in 
Mycobacteria to find the appropriate medium to use.  Also what may be relevant 
is that in the laboratory it takes up to six weeks to culture TB.  Not sure but 
this may be why you are not getting results.  
 
regards
Tony
 
 
 

Tony Reilly
Chief Scientist, Anatomical Pathology
Pathology Queensland-PA Laboratory
_
Clinical and Statewide Services Division| QueenslandHealth
 
Level 1, Building 15,Princess Alexandra Hospital
Ipswich Road,WOOLLOONGABBA  Qld4102
Ph: 07 3176 2412
Mob: 0402 139411
Fax: 07 3176 2930
Email: tony_rei...@health.qld.gov.au
Web:  www.health.qld.gov.au/qhcss/
 
 


 Gudrun Lang gu.l...@gmx.at 16/03/2010 1:14 am 
Hi all!

Can someone provide me with a procedure for selfmade Tb-control for
ZN-staining. 

I tried incubating some lungtissue (2x2x2 cm) in a solution with 3-6 drops
of bacteria-suspension for 3 hours and for 18 hours. Afterwards fixing in
NBF for 4 days.

I had no success. No stainable mycobacteria were found.



Bye

Gudrun

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Re: [Histonet] alcian blue van gieson stain

2010-03-14 Thread Anthony Reilly
Hi Margaret
 
You perform the Alcian Blue first but as with Movatt's pentachrome you need to 
treat the sections after AB with alcoholic ammonia for an hour to convert the 
AB to Monastral Blue as the AB is soluable in picric acid and the Monastral 
blue resistant. Let me know if you need a method
 
regards
Tony
 
 
 
 

Tony Reilly
Chief Scientist, Anatomical Pathology
Pathology Queensland-PA Laboratory
_
Clinical and Statewide Services Division| QueenslandHealth
 
Level 1, Building 15,Princess Alexandra Hospital
Ipswich Road,WOOLLOONGABBA  Qld4102
Ph: 07 3176 2412
Mob: 0402 139411
Fax: 07 3176 2930
Email: tony_rei...@health.qld.gov.au
Web:  www.health.qld.gov.au/qhcss/
 
 


 Perry, Margaret margaret.pe...@sdstate.edu 13/03/2010 12:30 am 
We want to try the double stain alcian blue Van gieson.  Do you stain for the 
alcian blue first and then the Van gieson?  We do both stains but I am unsure 
of how to put them together.
Margaret Perry
South Dakota State University

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RE: [Histonet] Double labeling with antibodies that need differentfixatives

2010-02-22 Thread Anthony Reilly
Hi Phebe
 
The first place to look when working up Antibodies is the Specification sheet 
from the manufacturer.  If you look at the BD sheet for their CD31 
Immunohistochemistry is recommended for Zinc fixed paraffin sections and 
acetone fixed frozeb sections but not recommended for formalin fixed paraffin 
sections.
 
regards
Tony
 
 

Tony Reilly
Chief Scientist, Anatomical Pathology
Pathology Queensland-PA Laboratory
_
Clinical and Statewide Services Division| QueenslandHealth
 
Level 1, Building 15,Princess Alexandra Hospital
Ipswich Road,WOOLLOONGABBA  Qld4102
Ph: 07 3176 2412
Mob: 0402 139411
Fax: 07 3176 2930
Email: tony_rei...@health.qld.gov.au
Web:  www.health.qld.gov.au/qhcss/
 
 


 Phebe Verbrugghe pverbrug...@meddent.uwa.edu.au 23/02/2010 2:09 pm 
Hi Adam,

Thanks a lot, might just give it a go on just formalin fixed tissue
first.

Phebe



From: Adam . [mailto:anonwu...@gmail.com] 
Sent: Tuesday, 23 February 2010 12:01 PM
To: Phebe Verbrugghe
Cc: histonet@lists.utsouthwestern.edu 
Subject: Re: [Histonet] Double labeling with antibodies that need
different fixatives


I have no idea if it would work with regular formalin. In my experience,
many antigens work as well in zinc buffered formalin without any antigen
retrieval as regular formalin with antigen retrieval. But really, you
just have to try it yourself.

On antibodies I've gotten this to work, I use commercially available
zinc buffered formalin which comes in gallon jugs for around $50. We
don't do any special processing. We plop our sample (bones) in zinc
formalin overnight at 4C, decalcify in EDTA or formic acid (only
necessary for bones), and then embed just like any other sample.

Adam


On Mon, Feb 22, 2010 at 9:45 PM, Phebe Verbrugghe
pverbrug...@meddent.uwa.edu.au wrote:


Hello Adam,

Thank you very much for this very useful information!
Do you know whether this would also work on tissue fixed with
formalin instead of zinc buffered formalin by any chance? 
Also, could you give me the recipe for the zinc formalin and can
I use a standard tissue processor for embedding in paraffin or should I
use a specific protocol manually and if so, which? 

Thanks!

Phebe



From: Adam . [mailto:anonwu...@gmail.com] 
Sent: Tuesday, 23 February 2010 10:52 AM
To: Phebe Verbrugghe
Cc: histonet@lists.utsouthwestern.edu 
Subject: Re: [Histonet] Double labeling with antibodies that
need different fixatives


Although I haven't tried it myself, others have gotten CD31 from
BD to work on FFPE tissue using the tyramide amplification system on
zinc buffered formalin fixed sections. I've generally had good luck with
zinc buffered formalin myself for many antigens so it may work for your
other one.

See http://www.ncbi.nlm.nih.gov/pubmed/19052548 

Just to be clear, they used zinc buffered formalin, which isn't
the same thing as zinc fixative.

Adam


On Mon, Feb 22, 2010 at 8:41 PM, Phebe Verbrugghe
pverbrug...@meddent.uwa.edu.au wrote:



Hi all,

I would like to do an immunofluorescent double labeling
with two
antibodies but 1 antibody works on acetone fixed frozen
tissue but not
on formalin fixed paraffin embedded tissue (CD31 BD
pharmingen 553370)
and the other one works on formalin fixed paraffin
embedded tissue but
not on acetone fixed frozen tissue. Is there any way I
could still do a
double labeling and how?
Also, does anyone have experience with zinc fixative? If
my antibody
works on formalin fixed tissue is it likely to also work
on zinc fixed
tissue?

Thank you very much in advance,

Phebe

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If not an intended recipient of this email, you must not copy, 

RE: [Histonet] Double labeling with antibodies that need differentfixatives

2010-02-22 Thread Anthony Reilly
Hi Phebe
 
The first place to look when working up Antibodies is the Specification sheet 
from the manufacturer.  If you look at the BD sheet for their CD31 
Immunohistochemistry is recommended for Zinc fixed paraffin sections and 
acetone fixed frozeb sections but not recommended for formalin fixed paraffin 
sections.
 
regards
Tony
 
 

Tony Reilly
Chief Scientist, Anatomical Pathology
Pathology Queensland-PA Laboratory
_
Clinical and Statewide Services Division| QueenslandHealth
 
Level 1, Building 15,Princess Alexandra Hospital
Ipswich Road,WOOLLOONGABBA  Qld4102
Ph: 07 3176 2412
Mob: 0402 139411
Fax: 07 3176 2930
Email: tony_rei...@health.qld.gov.au
Web:  www.health.qld.gov.au/qhcss/
 
 


 Phebe Verbrugghe pverbrug...@meddent.uwa.edu.au 23/02/2010 2:09 pm 
Hi Adam,

Thanks a lot, might just give it a go on just formalin fixed tissue
first.

Phebe



From: Adam . [mailto:anonwu...@gmail.com] 
Sent: Tuesday, 23 February 2010 12:01 PM
To: Phebe Verbrugghe
Cc: histonet@lists.utsouthwestern.edu 
Subject: Re: [Histonet] Double labeling with antibodies that need
different fixatives


I have no idea if it would work with regular formalin. In my experience,
many antigens work as well in zinc buffered formalin without any antigen
retrieval as regular formalin with antigen retrieval. But really, you
just have to try it yourself.

On antibodies I've gotten this to work, I use commercially available
zinc buffered formalin which comes in gallon jugs for around $50. We
don't do any special processing. We plop our sample (bones) in zinc
formalin overnight at 4C, decalcify in EDTA or formic acid (only
necessary for bones), and then embed just like any other sample.

Adam


On Mon, Feb 22, 2010 at 9:45 PM, Phebe Verbrugghe
pverbrug...@meddent.uwa.edu.au wrote:


Hello Adam,

Thank you very much for this very useful information!
Do you know whether this would also work on tissue fixed with
formalin instead of zinc buffered formalin by any chance? 
Also, could you give me the recipe for the zinc formalin and can
I use a standard tissue processor for embedding in paraffin or should I
use a specific protocol manually and if so, which? 

Thanks!

Phebe



From: Adam . [mailto:anonwu...@gmail.com] 
Sent: Tuesday, 23 February 2010 10:52 AM
To: Phebe Verbrugghe
Cc: histonet@lists.utsouthwestern.edu 
Subject: Re: [Histonet] Double labeling with antibodies that
need different fixatives


Although I haven't tried it myself, others have gotten CD31 from
BD to work on FFPE tissue using the tyramide amplification system on
zinc buffered formalin fixed sections. I've generally had good luck with
zinc buffered formalin myself for many antigens so it may work for your
other one.

See http://www.ncbi.nlm.nih.gov/pubmed/19052548 

Just to be clear, they used zinc buffered formalin, which isn't
the same thing as zinc fixative.

Adam


On Mon, Feb 22, 2010 at 8:41 PM, Phebe Verbrugghe
pverbrug...@meddent.uwa.edu.au wrote:



Hi all,

I would like to do an immunofluorescent double labeling
with two
antibodies but 1 antibody works on acetone fixed frozen
tissue but not
on formalin fixed paraffin embedded tissue (CD31 BD
pharmingen 553370)
and the other one works on formalin fixed paraffin
embedded tissue but
not on acetone fixed frozen tissue. Is there any way I
could still do a
double labeling and how?
Also, does anyone have experience with zinc fixative? If
my antibody
works on formalin fixed tissue is it likely to also work
on zinc fixed
tissue?

Thank you very much in advance,

Phebe

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Re: [Histonet] Polarizing filters

2009-09-17 Thread Anthony Reilly
I worked with a pathologist many years ago who would use one piece of 
polarising glass on the light source and wear his sunglasses.  It worked fine.
 
regards
Tony
 
 
 
 
Tony Reilly

Chief Scientist
Anatomical Pathology
Pathology Queensland
Level 1, Building 15
Princess Alexandra Hospital
Ipswich Rd, 
Woolloongabba Q 4102
Australia
Ph: 07 32402412
Fax:07 32402930
tony_rei...@health.qld.gov.au


 Eridana erid...@cox.net 18/09/2009 3:49 am 
You can use glass camera filters.  At the store they had a huge supply of 
polarizing filters.  I bought 2 for about $20 each that were the same brand, 
but not even the same diameter.  I put one on top of the slide and one on the 
light source and it worked great.  I also rotated the light source filter since 
it was too easy to bump the slide when trying to rotate the upper one.

It was really interesting to see all the non collagen that was positive in the 
staining but not when polarized.

Donna Harclerode HT,HTL,QIHC (ASCP),SLS 
Histology Core Manager 
UCSD, Dept of Pathology 
9500 Gillman Drive 
BSB 2010 
San Diego, CA 92071 
858 534 7438


Date: Wed, 16 Sep 2009 14:12:38 -0400 
From: Monfils, Paul pmonf...@lifespan.org 
Subject: RE: [Histonet] Polarizing filters 
To: histonet@lists.utsouthwestern.edu 
Message-ID: 
4ebff65383b74d49995298c4976d1d5e03835...@lsriexch1.lsmaster.lifespan.org 

Content-Type: text/plain;charset=iso-8859-1 

The polarizer and analyzer are identical filters, and either of them can be 
used 
in either location. One must be between the light source and the slide being 
viewed. The other must be between the slide being viewed and your eye or 
camera.  
I place one filter directly on top of my illuminator.  The other is in a filter 
slide in the microscope column, which can be pushed into the light beam or 
pulled out of it, but you can also place it directly on top of the slide. You 
rotate either filter to achieve the polarization effect.  I rotate the lower 
one 
since the other one is not accessible.  These filters cut down the light 
intensity substantially, so you should use them with maximum brightness of the 
illuminator, iris diaphram wide open, and with neutral density or any other 
kinds of filters removed from the light beam, including the blue filter if you 
normally use one.  Polarizing filters can be purchased at any camera store, and 
some science supply companies sell them.  Get good quality glass filters 
though, 
not cheap plastic ones. 

 -- 
 From: histonet-boun...@lists.utsouthwestern.edu on behalf of jstaruk 
 Sent: Thursday, September 10, 2009 4:46 PM 
 To: histonet@lists.utsouthwestern.edu 
 Subject: [Histonet] Polarizing filters 
 
 Does anyone know where I can find the two appropriate filters (lenses) 
 needed to polarize the congo red and Sirius red stains?  I have an Olympus 
 CH-2 that needs to be fitted.  I understand I need a polarizer lens and an 
 analyzer lens.  Are these two different lenses or the same lens, just in 
 different locations on the microscope? 
 
 Thank you 
 
 Jim 
 
 ___ 
 James E. Staruk HT(ASCP) 
  www.masshistology.com 
   www.nehorselabs.com 
 
 


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Re: [Histonet] water on slides?

2009-08-24 Thread Anthony Reilly
If your solutions are clean the cause may be that the level of the water wash 
station on your stainer is higher than the level of the subsequent alcohol 
container which means that some water will not be removed from the top of the 
slide.  This is common with running water washes on stainers as the water 
pressure will elevate the level.  A common artifact appears as a blue stripe 
down the slide caused by the water running down and removing the eosin.
 
regards
 
 
Tony Reilly

Chief Scientist
Anatomical Pathology
Pathology Queensland
Level 1, Building 15
Princess Alexandra Hospital
Ipswich Rd, 
Woolloongabba Q 4102
Australia
Ph: 07 32402412
Fax:07 32402930
tony_rei...@health.qld.gov.au


 Va Paula Sicurello vapat...@yahoo.com 25/08/2009 7:30 am 
I'm getting the same eosin bleeding and water on the slides.  I'm using Hemo-D 
and CitriSolv.  I have changed the reagents and am still getting the eosin 
bleeding, the water on the slide is a new phenomenon.

Any suggestions?


Paula Sicurello
VA Medical Center San Diego
Veterans Medical Research Foundation (VMRF) 
Core for Micro Imaging(C-MI)
3350 La Jolla Village Dr., MC151
San Diego, CA 92161
858-552-8585 x2397

C-MI for your imaging needs.


--- On Mon, 8/24/09, Angela Bitting akbitt...@geisinger.edu wrote:

 From: Angela Bitting akbitt...@geisinger.edu
 Subject: Re: [Histonet] water on slides?
 To: histonet@lists.utsouthwestern.edu, Tina J. Hayes tina.ha...@va.gov
 Date: Monday, August 24, 2009, 6:00 PM
 We are having a very similar problem
 too. We change our alcohols and Histoclear like mad, but are
 having eosin bleeding out of the sections. I'm starting to
 wonder if it is the mounting media on our glass
 coverslipper. I ordered new bottle gaskets, so I guess I'll
 see what happens then.
 
 Angela Bitting, HT(ASCP)
 Technical Specialist, Histology
 Geisinger Medical Center 
 100 N Academy Ave. MC 23-00
 Danville, PA 17822
 phone  570-214-9634
 fax  570-271-5916 
  
 No trees were hurt in the sending of this email
 However many electrons were severly inconvienienced!
 
 
  Hayes, Tina J. tina.ha...@va.gov
 8/24/2009 12:41 PM 
 We are having a problem with what seems to be water on our
 slides.  We
 have had very high humidity levels in the air.  It
 seems that we look at
 the slides before taking them to the pathology office, one
 pathologist
 reviews them and sees little or no water droplets, but as
 they sit and
 another pathologist reads them later, like the following
 day, the
 droplets are very apparent.
 
  
 
 We use Clearite-3.  We have no xylene in our
 lab.  We also coverslip
 with Permount.
 
  
 
 Is it possible that the clearite-3 and/or Permount is
 absorbing moisture
 from the atmosphere to the slides?
 
 And if so, do you have any suggestions for combating this
 issue?
 
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 http://lists.utsouthwestern.edu/mailman/listinfo/histonet 
 
 
 
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 Access to this message by anyone else is unauthorized. If
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Re: [Histonet] Pathology to OR Communication System

2009-06-22 Thread Anthony Reilly
Hi Luke
 
A simple cheap solution would be to buy telephones for the OR and the lab that 
have speaker phone capabilities.  No expensive purchase cost or installation 
required.
 
regards
Tony
 
 
 
 
Tony Reilly

Chief Scientist
Anatomical Pathology
Pathology Queensland
Level 1, Building 15
Princess Alexandra Hospital
Ipswich Rd, 
Woolloongabba Q 4102
Australia
Ph: 07 32402412
Fax:07 32402930
tony_rei...@health.qld.gov.au


 Perkocha, Luke luke.perko...@ucsf.edu 23/06/2009 2:41 am 
Hello All,

We have a very old speakerphone system that we use to call from the 
pathologist's office in to our operating rooms to discuss frozen section 
diagnoses with the surgeons. Both sides are yelling and straining to hear and 
we're concerned about the risk for miscommunication. We can't go into the OR 
directly, since Pathology and the OR are too far apart physically.

We're looking for some sort of telephone-based communications system, perhaps 
with a speaker and microphone that can be mounted near the surgeon, so that 
when we call into the OR with the frozen section diagnosis, it can be switched 
to speaker and the call can be continued with direct and audible communication 
between the pathologist on the phone in his/her office and the surgical team at 
the head of the operating table.

Does anyone out there have a system like this?

Do you know of a commercial vendor who makes something that would work?

We tried an expensive Polycom system meant for conference calls, but its 360 
degree microphones picked up too much background noise in the OR.

It seems like it should be a simple Radio Shack project, but we're all 
techno-challenged.

Any help would be appreciated. Thanks.

Luke Perkocha
luke.perko...@ucsf.edumailto:luke.perko...@ucsf.edu

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Re: [Histonet] (no subject)

2009-04-14 Thread Anthony Reilly
I have used DAKO Target Retrieval in the past and it is definitely possible to 
re-use the solution.  The important thing to do is to check the pH each day 
before use as this is the best indicator that the solution needs to be changed. 
 It has bee an while since I used it but  from my shaky memory you should get 
at least a week from the solution.
 
regards
 
 
Tony Reilly

Chief Scientist
Anatomical Pathology
Pathology Queensland
Level 1, Building 15
Princess Alexandra Hospital
Ipswich Rd, 
Woolloongabba Q 4102
Australia
Ph: 07 32402412
Fax:07 32402930
tony_rei...@health.qld.gov.au


 jeff jlhow...@yrmc.org 15/04/2009 1:55 am 
Is anyone using their target retrieval for dako more than 1 time?

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Re: FW: [Histonet] (no subject)

2009-04-14 Thread Anthony Reilly
As per Young's response, I have never diluted the solution further but found 
that if there was some drop in the level of the solution due to evaporation it 
could be topped up with deionised water as long as the pH was not changed.  
This was on the advice of the DAKO rep at the time.
 
regards
 
 
Tony Reilly

Chief Scientist
Anatomical Pathology
Pathology Queensland
Level 1, Building 15
Princess Alexandra Hospital
Ipswich Rd, 
Woolloongabba Q 4102
Australia
Ph: 07 32402412
Fax:07 32402930
tony_rei...@health.qld.gov.au


 Young Kwun kw...@email.cs.nsw.gov.au 15/04/2009 1:29 pm 


I also used Dako's Target Retrieval buffer in the past and it was also
possible to dilute further up to 1:20 or 1:40 (instead of 1:10) with good
results.

Young


-Original Message-
From: histonet-boun...@lists.utsouthwestern.edu 
[mailto:histonet-boun...@lists.utsouthwestern.edu] On Behalf Of Anthony
Reilly
Sent: Wednesday, 15 April 2009 10:31 AM
To: histonet@lists.utsouthwestern.edu; jeff
Subject: Re: [Histonet] (no subject)

I have used DAKO Target Retrieval in the past and it is definitely possible
to re-use the solution.  The important thing to do is to check the pH each
day before use as this is the best indicator that the solution needs to be
changed.  It has bee an while since I used it but  from my shaky memory you
should get at least a week from the solution.

regards


Tony Reilly

Chief Scientist
Anatomical Pathology
Pathology Queensland
Level 1, Building 15
Princess Alexandra Hospital
Ipswich Rd, 
Woolloongabba Q 4102
Australia
Ph: 07 32402412
Fax:07 32402930
tony_rei...@health.qld.gov.au 


 jeff jlhow...@yrmc.org 15/04/2009 1:55 am 
Is anyone using their target retrieval for dako more than 1 time?

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Re: [Histonet] Strange circles in IHC slides

2009-04-02 Thread Anthony Reilly
Hi
 
Looking at the images this appears to be the prozone effect which is caused by 
the primary antibody concentration being too high and has been well reported in 
both immunohistochemistry, immunology and serology articles.  Do a google serch 
for prozone phenomenon and you will find an explanation of the theory involved. 
   The classic feature are the circular areas which are unstained and this is 
reinforced in the images by the amount of background staining in the areas that 
are stained.  Try titrating your primary out and I am sure will eliminate the 
problem.
 
regards
 
 
Tony Reilly

Chief Scientist
Anatomical Pathology
Pathology Queensland
Level 1, Building 15
Princess Alexandra Hospital
Ipswich Rd, 
Woolloongabba Q 4102
Australia
Ph: 07 32402412
Fax:07 32402930
tony_rei...@health.qld.gov.au


 V. Neubert histonet.nos...@vneubert.com 3/04/2009 2:12 am 
Hello,

I really have some real links to real pictures of real relevance of the 
real histonet list. Really promised.

http://img12.imageshack.us/img12/8513/ts0402162049.jpg 
http://img13.imageshack.us/img13/6514/ts0402162104.jpg 

So, has ever anyone experienced sth. like this?
My conjugate control (every step except the antibody) was fine, nothing 
to be seen about DAB and no circles at all.

I used Shandon single-use coverplates, sterile buffer, fresh antibody 
aliquots. Any idea?

Thanks,

V. Neubert

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[Histonet] Calcium salts

2009-03-30 Thread Anthony Reilly
Hello
 
I am trying to differentiate Calcium Phosphate from Calcium Carbonate which 
both stain with the von Kossa method.  Is there a pretreatment for which only 
one is soluble that could be used to differentiate the 2 components.
 
thanks
 
 
Tony Reilly

Chief Scientist
Anatomical Pathology
Pathology Queensland
Level 1, Building 15
Princess Alexandra Hospital
Ipswich Rd, 
Woolloongabba Q 4102
Australia
Ph: 07 32402412
Fax:07 32402930
tony_rei...@health.qld.gov.au


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Re: [Histonet] overseas jobs

2009-02-26 Thread Anthony Reilly
Hello Joe
 
This is an interesting question following on from all of the discussion 
recently about uncertified techs.  In Australia you need tertiary 
qualifications to work in a technical position in Histology.  Histologists are 
regarded and paid at the same level as all other staff working in medical 
pathology laboratories.  There are 2 levels of staff with those people with an 
Associate Diploma called Laboratory Technicians and those with a degree called 
Medical Scientists ( a little extra pay) generally, though the names can vary a 
little from region to region.  Most Scientists have done a B.Sc in Medical 
Laboratory Science which involves studying Histology, Haematology, 
Biochemistry, Blood Transfusion Medicine,  Microbiology, Immunology and 
Molecular Studies and qualifies the graduate to work in any of these fields and 
I have known a number of people including my wife who have changed vocation 
more than once in their working life.  She started in Microbiology had 8 years 
in Histology including EM moved to Haematology for a few years and now runs a 
smaller multiskilled laboratory where she does Haematology, Blood Banking, 
Biochemistry and limited Microbiology on a daily basis.  The first 7 years of 
my working life were spent in Histology during the day and on the on-call 
roster for nights and weekends to do Haematology, Blood Banking, Biochemistry 
and  Microbiology.  Hence the equal status with other disciplines.
 
To get back to your original question she would need firstly to get a work visa 
as in my organisation (public government laboratory) we are not permitted to 
interview anybody who does not have a work visa and we can not arrange for 
people to get them.  Secondly she would need to get her qualifications assessed 
by either a government body or our institute
the Australian Institute of Medical Scientists (AIMS).  Their website can be 
found on the net.  If she is graded at degree level she can be employed as a 
Medical Scientist, if assessed at Diploma level employed as  a Technician but 
if it is assessed below that level such as a certificate she could only be 
employed as a Laboratory Assistant. ( much less pay)
 
I hope this is useful.  
P.S. I always enjoy your insightful contributions to the Histonet.
 
regards
 
 
Tony Reilly

Chief Scientist
Anatomical Pathology
Pathology Queensland
Level 1, Building 15
Princess Alexandra Hospital
Ipswich Rd, 
Woolloongabba Q 4102
Australia
Ph: 07 32402412
Fax:07 32402930
tony_rei...@health.qld.gov.au


 JoeNocito jnoc...@satx.rr.com 27/02/2009 9:41 am 
Howdy Histo land,

I'm posting this message for one of my current students. She graduates in
August from the Histology program and wants to know what the job market is
overseas, especially in the U.K. Any ideas? What will she have to do to be
able to work in Europe or Australia? Thanks for your time.



JTT

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Re: [Histonet] equation problem PLEASE help

2009-01-07 Thread Anthony Reilly
Hello Eva
 
Put simply
 

1nmol is 10-9 moles 
Therefore 10nmol is 10-8 moles
1 mole = 1,064g
Therefore 10-8 moles = 0.1064gor 0.01064mg
Therefore your working solution of 10nmol/ml = 0.01064mg/ml
 
Your stock solution is 1mg/ml
Therefore your dilution factor is 1.0   =  
94 (93.984962 exactly)
0.01064
 
Therefore you can add 1ml stock to 93ml of diluent to get your desired 
concentration..
 
 I hope this is useful
 
regards
 
 
 
Tony Reilly

Chief Scientist
Anatomical Pathology
Pathology Queensland
Level 1, Building 15
Princess Alexandra Hospital
Ipswich Rd, 
Woolloongabba Q 4102
Australia
Ph: 07 32402412
Fax:07 32402930
tony_rei...@health.qld.gov.au


 e...@georgetown.edu 8/01/2009 7:46 am 
Good afternoon,
I am hoping someone out there will take pity on a mathematically challenged 
individual such as myself. I have been trying for hours to wrap my head around 
this equation and am now getting to the point where I am more confused than 
ever. Please help me.
The protocol calls for 10nmol of a substance per 1ml needed. It comes in a 
1mg/ml solution and has a molecular weight of 1064g/mol. How do I do this? If 
for example I needed 2ml of the solution...
The clearer the explanation the better. I really want to understand the 
calculation not just have an answer. PLEASE HELP ME.
Thank you,
Eva

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Re: [Histonet] equation problem PLEASE help

2009-01-07 Thread Anthony Reilly
Hello Eva
 
Unfortunately some of the script did not transfer in the original mail and 10-9 
should read 10 to the minus 9 as the superscript was lost.  The same for 10-8.  
Also there should have been a division line between 1.0 and 0.01064 in the 
calculation.  I hope this helps.
 
regards
 
Tony Reilly

Chief Scientist
Anatomical Pathology
Pathology Queensland
Level 1, Building 15
Princess Alexandra Hospital
Ipswich Rd, 
Woolloongabba Q 4102
Australia
Ph: 07 32402412
Fax:07 32402930
tony_rei...@health.qld.gov.au

 Anthony Reilly tony_rei...@health.qld.gov.au 8/01/2009 12:39 pm 
Hello Eva

Put simply


1nmol is 10-9 moles 
Therefore 10nmol is 10-8 moles
1 mole = 1,064g
Therefore 10-8 moles = 0.1064gor 0.01064mg
Therefore your working solution of 10nmol/ml = 0.01064mg/ml

Your stock solution is 1mg/ml
Therefore your dilution factor is 1.0   =  
94 (93.984962 exactly)
0.01064

Therefore you can add 1ml stock to 93ml of diluent to get your desired 
concentration..

I hope this is useful

regards



Tony Reilly

Chief Scientist
Anatomical Pathology
Pathology Queensland
Level 1, Building 15
Princess Alexandra Hospital
Ipswich Rd, 
Woolloongabba Q 4102
Australia
Ph: 07 32402412
Fax:07 32402930
tony_rei...@health.qld.gov.au 


 e...@georgetown.edu 8/01/2009 7:46 am 
Good afternoon,
I am hoping someone out there will take pity on a mathematically challenged 
individual such as myself. I have been trying for hours to wrap my head around 
this equation and am now getting to the point where I am more confused than 
ever. Please help me.
The protocol calls for 10nmol of a substance per 1ml needed. It comes in a 
1mg/ml solution and has a molecular weight of 1064g/mol. How do I do this? If 
for example I needed 2ml of the solution...
The clearer the explanation the better. I really want to understand the 
calculation not just have an answer. PLEASE HELP ME.
Thank you,
Eva

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Re: [Histonet] Slide drying

2008-12-22 Thread Anthony Reilly
Hi Erin
 
While the request from your pathologists seems unreasonable from my experience 
the following steps will give the best results.  Use a rapid drying mountant 
many of which are on the market.  Consult your local suppliers.  Dry in an 
incubator as you have been doing but when you remove from the incubator allow 
the slides to cool before filing or even sorting into piles.  The mountant may 
be dry but the heat will make it sticky gluing the slides together.  Just think 
of new bitumen on a very hot day.
 
All the best.
 
 
 
Tony Reilly

Chief Scientist
Anatomical Pathology
Pathology Queensland
Level 1, Building 15
Princess Alexandra Hospital
Ipswich Rd, 
Woolloongabba Q 4102
Australia
Ph: 07 32402412
Fax:07 32402930
tony_rei...@health.qld.gov.au


 Martin, Erin erin.mar...@ucsf.edu 23/12/2008 5:06 am 
Hello everyone,

I was asked to find out how to dry slides quickly.  They are glass coverslipped 
in an automated coverslipper at the reference lab we use and the our docs want 
them filed in less than 12 hours from the time they are coverslipped.   We have 
been putting them in a 125 degree C convection oven for a few hours but the 
slides still get all stuck together in the file.  They will not consider film 
coverslipping. 

Does anyone else file this quickly?  I am grateful for any suggestions!

Erin Martin UCSF Dermatopathology


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