Re: [Histonet] Ventana Retic problems
We have had the same problem our solution was not the second but the wash, it for a bad too quickly so we don't make a full carboy and let it sit for a week, we make fresh wash almost daily, ESPECIALLY when we have a retic. Our stains look great daily with fresh wash solution. You may try that, hope it helps. Curt Sent from my Verizon, Samsung Galaxy smartphone Original message From: Jeffrey Robinson via HistonetDate: 6/14/17 4:01 PM (GMT-08:00) To: donna mihalik rossi Cc: histonet@lists.utsouthwestern.edu Subject: Re: [Histonet] Ventana Retic problems Hi Donna- I have been dealing with these same exact issues for 3 1/2 years now so I think I have achieved "expert status" in dealing with this problem. First, I'll give you my current protocol. When all things are working smoothly, it produces a nice stain. But it is very frustrating when it starts to "fade." We cut all retics at 5. Thinner cuts will definitely look lighter. Protocol: warmup slide: 47 degrees C. Oxidizer:4 minutes Decolorizer: 4 minutes Sensitizer: 8 minutes Optimize Counterstain Intensity: 4 Minutes I have gone around and around with Ventana on decontamination problems with this instrument. I was performing full decontamination runs every month. My rep finally said to just decon the bulk wash carboy and the wash bottle on the instrument when fading begins to show. Ventana claims there will be a new wash out this year that will hopefully take care of the problem once and for all but no one at Ventana can give me a release date on that. In the meantime, this is what I do: Daily: run the "Purge Wash" function test 3 times in the morning before running any slides. Be sure to run the "Purge" function and not the "Prime" function. When loading slides, put all of your retic slides on after everything else (after the GMS, etc., slides). When staining starts to fade: after ruling out "thin cuts" and other obvious problems it is time for decon. The fading will show first on the patient tissue (the control may still look OK). Here is my current decon protocol: I use the Lysol IC decon solution. I have an extra 6 gallon carboy and I leave some made up (diluted) so that it is ready to go. Put some decon solution on a 4X4 guaze and wipe the dispenser tip underneath the top (lift lid up for access). Dump the wash solution in the wash bottle on the instrument. Rinse out with DI water. Fill with decon solution. Swish solution inside bottle. Replace bottle (on instrument). Run "Purge Wash" function test (3 times). After Purge #3, let the solution sit in the lines for at least 15 minutes (the longer the better). When you are ready to proceed, rinse bulk bottle well several times and replace with DI water. Run "Purge Wash" 3 more times. Time is not a factor here so you can just run them one after another. After the third purge, replace the DI with BM SS wash. Run "Purge Wash" function test 3 more times. That's it. I find I need to run this procedure about once a month. Additionally, I decon the 5 gallon bulk wash carboy EVERY TIME I make up a new batch. It doesn't take long (I just let the decon solution sit for 15 minutes) and then when I do need to do the modified decon on the instrument I do not need to worry about the bulk carboy. I hope this helps- it takes a little time but it does seems to help with the retic stain intensity. Jeff Robinson, Senior Histotechnologist (HT, HTL), Sierra Pathology Lab, Clovis, CA. -Original Message- From: donna mihalik rossi via Histonet [mailto:histonet@lists.utsouthwestern.edu] Sent: Wednesday, June 14, 2017 1:45 PM To: histonet Subject: [Histonet] Ventana Retic problems Hi Histonetters! We are experiencing sporadic staining of retic fibers from our Ventana Benchmark machines. We have 2 machines and are having the same problem on both. The machines were both decontaminated 2 weeks ago with all new solutions being made. The fibers are not crisp and are disconnected. Our control tissue is at the top of the slide with the patient tissue at the bottom. It appears that the control is staining better than the patient tissue but still is not crisp. We have tried different lots with the same result. Any comments before we consult Ventana? Your help would be appreciated. Thanks, Donna Rossi, PSU ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet This email and attachments may contain PHI that is privileged and confidential and is not intended for any unauthorized person. If you, the reader, are not the intended recipient you are hereby notified that any dissemination, distribution or copying of this communication is strictly prohibited. Do not read the email
[Histonet] Fixation and IHC
Hi histonetters! Can anyone tell me what, if any, guidelines there are for fixation time for animal tissue with potential subsequent IHC stains. I am very familiar with CAP guidelines for receptor testing with breast cases, but I can't seem to find much on IHC for animal tissue. Thanks, Cristi ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
Re: [Histonet] Ventana Retic problems
Hi Donna- I have been dealing with these same exact issues for 3 1/2 years now so I think I have achieved "expert status" in dealing with this problem. First, I'll give you my current protocol. When all things are working smoothly, it produces a nice stain. But it is very frustrating when it starts to "fade." We cut all retics at 5. Thinner cuts will definitely look lighter. Protocol: warmup slide: 47 degrees C. Oxidizer:4 minutes Decolorizer: 4 minutes Sensitizer: 8 minutes Optimize Counterstain Intensity: 4 Minutes I have gone around and around with Ventana on decontamination problems with this instrument. I was performing full decontamination runs every month. My rep finally said to just decon the bulk wash carboy and the wash bottle on the instrument when fading begins to show. Ventana claims there will be a new wash out this year that will hopefully take care of the problem once and for all but no one at Ventana can give me a release date on that. In the meantime, this is what I do: Daily: run the "Purge Wash" function test 3 times in the morning before running any slides. Be sure to run the "Purge" function and not the "Prime" function. When loading slides, put all of your retic slides on after everything else (after the GMS, etc., slides). When staining starts to fade: after ruling out "thin cuts" and other obvious problems it is time for decon. The fading will show first on the patient tissue (the control may still look OK). Here is my current decon protocol: I use the Lysol IC decon solution. I have an extra 6 gallon carboy and I leave some made up (diluted) so that it is ready to go. Put some decon solution on a 4X4 guaze and wipe the dispenser tip underneath the top (lift lid up for access). Dump the wash solution in the wash bottle on the instrument. Rinse out with DI water. Fill with decon solution. Swish solution inside bottle. Replace bottle (on instrument). Run "Purge Wash" function test (3 times). After Purge #3, let the solution sit in the lines for at least 15 minutes (the longer the better). When you are ready to proceed, rinse bulk bottle well several times and replace with DI water. Run "Purge Wash" 3 more times. Time is not a factor here so you can just run them one after another. After the third purge, replace the DI with BM SS wash. Run "Purge Wash" function test 3 more times. That's it. I find I need to run this procedure about once a month. Additionally, I decon the 5 gallon bulk wash carboy EVERY TIME I make up a new batch. It doesn't take long (I just let the decon solution sit for 15 minutes) and then when I do need to do the modified decon on the instrument I do not need to worry about the bulk carboy. I hope this helps- it takes a little time but it does seems to help with the retic stain intensity. Jeff Robinson, Senior Histotechnologist (HT, HTL), Sierra Pathology Lab, Clovis, CA. -Original Message- From: donna mihalik rossi via Histonet [mailto:histonet@lists.utsouthwestern.edu] Sent: Wednesday, June 14, 2017 1:45 PM To: histonet Subject: [Histonet] Ventana Retic problems Hi Histonetters! We are experiencing sporadic staining of retic fibers from our Ventana Benchmark machines. We have 2 machines and are having the same problem on both. The machines were both decontaminated 2 weeks ago with all new solutions being made. The fibers are not crisp and are disconnected. Our control tissue is at the top of the slide with the patient tissue at the bottom. It appears that the control is staining better than the patient tissue but still is not crisp. We have tried different lots with the same result. Any comments before we consult Ventana? Your help would be appreciated. Thanks, Donna Rossi, PSU ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet This email and attachments may contain PHI that is privileged and confidential and is not intended for any unauthorized person. If you, the reader, are not the intended recipient you are hereby notified that any dissemination, distribution or copying of this communication is strictly prohibited. Do not read the email but instead reply to the sender and destroy the message and any attachments. Thank you. ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
[Histonet] Ventana Retic problems
Hi Histonetters! We are experiencing sporadic staining of retic fibers from our Ventana Benchmark machines. We have 2 machines and are having the same problem on both. The machines were both decontaminated 2 weeks ago with all new solutions being made. The fibers are not crisp and are disconnected. Our control tissue is at the top of the slide with the patient tissue at the bottom. It appears that the control is staining better than the patient tissue but still is not crisp. We have tried different lots with the same result. Any comments before we consult Ventana? Your help would be appreciated. Thanks, Donna Rossi, PSU ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
Re: [Histonet] Histologist In Oregon
HI Rueben. There is 2 HT positions in Salem if you are interested. Calleven for details 407-307-8604 Sent from Yahoo Mail on Android On Wed, Jun 14, 2017 at 5:17 AM, RC via Histonetwrote: Hey fellow histologists! Top of the morning. I’m looking for histology positions in the state of Oregon. 16 years of experience covering all facets of histology (R, Drug Discovery, Clinical Diagnostic, Reference) If any of your laboratories are in need, please contact me. Grazie! Rueben Carter ___ 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] Installing a new auto stainer
Hello, I am a small lab that has just relocated to a new building. As a part of the new lab construction we are installing our first auto-stainer. The plumber is concerned about any required permitting or precautions regarding back flow of reagents. I haven’t been able to find any information either way, because most labs have building operations management teams handle that end. Has anyone installed a new auto-stainer that knows if any special permitting, etc. is required? Thanks so much and feel free to contact me, Katie Riley Technical Supervisor of Dermatopathology Puyallup Dermatology Clinic ka...@puyallupderm.com ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
[Histonet] 3D plastic
Hello Histonet, I've been asked to section 3D plastic with tissue attached. I will be finding out what type of plastic it is. Has anyone done this? Will I still be able to use paraffin? Thanks for any information. Mary Lou Norman NYS College of Veterinary Medicine Cornell University ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
Re: [Histonet] Microwave processors
We are quite happy with Milestone Histos3 for processing our prostate and bladder biopsies quickly. Lester J. Raff, MD MBA UroPartners Medical Director Of Laboratory 2225 Enterprise Dr. Suite 2511 Westchester, Il 60154 Tel: 708-486-0076 Fax: 708-492-0203 -Original Message- From: Charles Riley via Histonet [mailto:histonet@lists.utsouthwestern.edu] Sent: Wednesday, June 14, 2017 8:39 AM To: Histo List Subject: [Histonet] Microwave processors Does anyone have any suggestions for microwave processing units? My lab processes about 110 blocks max a day from GI biopsies to breast tissue on size Sent from my iPhone ___ 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] Microwave processors
Charles, Milestone Medical http://www.milestonemed.com/ The processors are great. Easy to operate and use minimal chemicals based on the protocols you select. H and IHC are very good. Check out the various product offerings to see which unit will meet your needs best. Walter Benton HT(ASCP)QIHC Lab Operations Manager Chesapeake Urology Associates 806 Landmark Drive, Suite 127 Glen Burnie, MD 21061 410-768-5961 (Lab) 410-768-5965 (Fax) Chesapeakeurology.com Voted a Best Place to Work by Baltimore and Modern Healthcare Magazines. -Original Message- From: Charles Riley via Histonet [mailto:histonet@lists.utsouthwestern.edu] Sent: Wednesday, June 14, 2017 9:39 AM To: Histo ListSubject: [Histonet] Microwave processors Does anyone have any suggestions for microwave processing units? My lab processes about 110 blocks max a day from GI biopsies to breast tissue on size Sent from my iPhone ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet CONFIDENTIALITY NOTICE: The information contained in this electronic message is intended solely for the personal and confidential use of the designated recipient(s) named above and may contain information that is protected from disclosure under applicable law. If you are not the intended recipient, or the employee or agent responsible for delivering it to the intended recipient, you are hereby notified that any dissemination, distribution or copying of this transmission is strictly prohibited. If you have received this transmission in error, please notify the transmitting person/department immediately by email or telephone (410) 581-5881 and delete the message without making a copy. ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
[Histonet] Microwave processors
Does anyone have any suggestions for microwave processing units? My lab processes about 110 blocks max a day from GI biopsies to breast tissue on size Sent from my iPhone ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
[Histonet] Paraffin histology with Muscle
Dear all, Does anyone have optimization tips for using paraffin histology with muscle? We do have access to a cryostat to do frozen histology, but it's not our lab's thus we have to pay to use it. We do have all the materials necessary for paraffin-based histology though. I've noticed that muscle can be more difficult to use with paraffin. Do you guys have any processing or cutting tips? Thanks! Lucas Olson ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
[Histonet] H + E Staining protocols
Dear All, There are many variants to the standard H + E protocol. I'm seeking to optimize the current protocol our laboratory uses (pasted below). Do you guys have any suggestions of optimization (e.g. cutting down on the long water rinse after hematoxylin and increasing bluing reagent time)? Or if you have protocols that you'd think would be better please let me know. Our lab deals primarily with bone/cartilage/muscle. Our current protocol: Staining Preparation 1. After sectioning samples, dry in oven. Time Temp C Overnight 37 2-3 hours 45 30 minutes 55 Deparaffinization 1. Remove paraffin with xylene a. 2 minutes xylene b. 2 minutes in fresh xylene c. 2 minutes in fresh xylene d. 2 minutes in fresh xylene 2. Remove excess xylene 3. Rehydrate samples a. 1 minute absolute EtOH b. 1 minute different bucket of absolute EtOH c. 30 seconds in 95% absolute EtOH d. 45 seconds in 70% EtOH 4. Rinse with water for 1 minute Hematoxylin and Eosin Staining 1. Stain in hematoxylin (VWR 95057-858) for 5-10 minutes a. Optimized time for calvarium bone: 10 minutes b. Solution may be filtered to remove oxidized particles 2. Rinse in running tap water for 20 minutes 3. Decolorize in Clarifier 1 (1 second) a. Longer time (up to 3 seconds) will yield a lighter color. Discard after each use. 4. Immerse in VWR Bluing Reagent (30 sec- 1 minute) a. Dilute 25mL bluing reagent in 475 mL ultrapure H2O to working stock b. Optimized time for calvarium bone: 90 seconds 5. Rinse well in tap water (5 minutes) 6. Rinse in 95% ETOH (30 sec- 1 minute) 7. Counterstain in Eosin (30 sec- 90 sec) a. Optimized time for calvarium bone: 30 seconds 8. Dehydrate a. ETOH 95% (3 minutes) b. ETOH 95% (3 minutes) c. ETOH 100% (3 minutes) d. ETOH 100% (3 minutes) 9. Clear in Xylene (5 minutes) 10. Clear in new Xylene (5 minutes) 11. Mount with Cytoseal in fume hood and coverslip Thanks! Lucas Olson ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet
[Histonet] Histologist In Oregon
Hey fellow histologists! Top of the morning. I’m looking for histology positions in the state of Oregon. 16 years of experience covering all facets of histology (R, Drug Discovery, Clinical Diagnostic, Reference) If any of your laboratories are in need, please contact me. Grazie! Rueben Carter ___ Histonet mailing list Histonet@lists.utsouthwestern.edu http://lists.utsouthwestern.edu/mailman/listinfo/histonet