Name: normal and malignant muscle cell transplantation into immune compromised adult zebrafish
Uploaded: 2014-12-26T15:00:00.000+00:00
Duration: 9 min 39 s
Description: Watch this Scientific Journal Video about Normal and Malignant Muscle Cell Transplantation into Immune Compromised Adult Zebrafish at JoVE.com

This work is supported by Alex&#8217;s Lemonade Stand Foundation (D.M.L.), American Cancer Society (D.M.L.), the MGH Howard Goodman Fellowship (D.M.L.), and US National Institutes of Health grants R24OD016761 and 1R01CA154923 (D.M.L.). CNY Flow Cytometry Core and Flow Image Analysis, shared instrumentation grant number 1S10RR023440-01A1. I.M.T. is funded by a fellowship from the Portuguese Foundation for Science and Technology (Funda&#231;&#227;o para a Ci&#234;ncia e Tecnologia &#8211; FCT). Q.T. is funded by the China Scholarship Council. We thank Angela Volorio for her helpful comments and advice.

All animal procedures were approved by Massachusetts General Hospital Subcommittee on Research Animal Care, under protocol #2011N000127.
Section 1. Skeletal Muscle Cell Transplantation into Adult rag2E450fs Homozygous Mutant Zebrafish
1. Preparation of Adult Zebrafish Donor Skeletal Muscle Cells
<ol>
	<li>Obtain transgenic adult zebrafish that have fluorescently labeled muscle. In this experiment, 30 &#945;-actin-RFP donor fish25 were utilized to transplant 1 x 106 cells per recipient fish.</li>
	<li>Sacrifice donor zebrafish in 1.6 mg/ml tricaine methanesulfonate (MS222) for 10 min or until no operculum movement is evident.</li>
	<li>Place donor fish on an absorbent paper towel and excise the dorsal muscle using a clean razor blade. The cut should be made near the anus at a 45&#176; angle to maximize tissue collection (as noted in Figure 1A). Place dissected tissue into a clean 10 cm Petri dish.</li>
	<li>Add 500 &#956;l suspension buffer (pre-chilled 0.9x Phosphate Buffer Saline (PBS) supplemented with 5% Fetal Bovine Serum (FBS)) to the dissected tissue. Up to 10 donor zebrafish can be placed together in this volume.</li>
	<li>Mince the tissue with a razor blade &#62;20 times until cells are in a uniform suspension. The entire dorsal musculature is homogenized including skin, bones and fins. Add 2 ml of suspension buffer. Using a 5 ml pipette, triturate the cell suspension &#8805;20 times to dissociate cells.</li>
	<li>Filter the cell suspension through a 40 &#956;m mesh strainer into a 50 ml conical tube placed on ice.</li>
	<li>Wash the Petri dish with an additional 2.5 ml of suspension buffer to collect remaining tissue and filter through the same strainer and conical tube, to a final volume of 5 ml (10 donor fish can be used per isolate). 
	NOTE: Skin, bones and fins will be excluded following filtration.</li>
	<li>If applicable, combine similar suspensions into the same conical tube.</li>
	<li>Count the total number of viable cells using trypan blue dye and a hemocytometer.</li>
	<li>Reserve 500 &#956;l for flow cytometry, if desired (optional, step 2).</li>
	<li>Centrifuge cell suspension at 1,000 x g, for 10 min, at 4 &#176;C.</li>
	<li>Discard supernatant and resuspend cells at 3.33 x 105 cells/&#956;l (0.9x PBS + 5% FBS). In total, 3 &#956;l will be injected per recipient fish for a total of 1 x 106 cells per recipient (step 3). 
	NOTE: Less than 3 &#956;l of cell suspension should be transplanted into the recipient fish. If cell number is limiting, as low as 5 x 104 cells per recipient can lead to successful engraftment (Table 1).</li>
</ol>
2. Flow Cytometry Analysis of Donor Skeletal Muscle Cell Preparation (Optional)
<ol>
	<li>Isolate muscle from a wild type, non-transgenic fish as outlined in step 1.1. This sample serves as the negative control and is useful for setting Flow Cytometry gates.</li>
	<li>Add an appropriate viability dye. For example, add 5 &#956;l of stock DAPI solution (500 ng/&#956;l) to 500 &#956;l of muscle preparation. Vortex slightly prior to analysis. Acquire 5 x 103 to 1 x 104 events. Analyze wild type control samples first to place gates followed by analysis of muscle cells isolated from transgenic fish. 
	NOTE: Flow cytometry analysis is usually performed within 1 hr after muscle tissue dissection, during which time the dissected cells retain more than 60% viability (Figure 2). Cells should be kept on ice at all times. Total cell viability can be re-assessed prior to transplantation using trypan blue dye and a hemocytometer.</li>
</ol>
3. Intramuscular Transplantation of Skeletal Muscle Cells into Adult rag2 Homozygous Mutant Zebrafish
<ol>
	<li>Clean a 10 &#956;l 26S G micro-syringe by drawing in and expelling 10% bleach solution (5 times), followed by 70% ethanol (5 times), and then followed by suspension buffer (0.9x PBS + 5% FBS, 10 times).</li>
	<li>Anesthetize 2-4 month old homozygous rag2 mutant fish or wild type recipient fish (as controls) by adding single drops of tricaine methanesulfonate (MS222, 4 mg/ml stock solution) into a Petri dish containing the fish in system water until operculum movements slow and fish are still. 
	NOTE: Dose of tricaine anesthesia will depend on age and size of recipient zebrafish.</li>
	<li>Place anesthetized recipient zebrafish on a damp paper towel or sponge, with the left side facing up.</li>
	<li>Insert the syringe needle into the latero-dorsal musculature (refer to Figure 1A). Ensure that injections are performed at a 45&#176; angle. Inject 3 &#956;l of the cell suspension (prepared in step 1.12) per fish for a total of 1 x 106 cells per recipient.</li>
	<li>Carefully transfer injected zebrafish into a clean tank using a plastic spoon to recover.</li>
	<li>Assess recipient zebrafish for engraftment rates at 10, 20, 30 days post-transplantation by imaging anesthetized fish under bright field and epifluorescence microscopy.</li>
</ol>


Section 2. Embryonal Rhabdomyosarcoma (ERMS) Transplantation into Adult Homozygous rag2 Mutant Zebrafish
4. DNA Microinjection of Zebrafish Embryos
<ol>
	<li>Linearize the rag2-kRASG12D plasmid7 by digesting 10 &#956;g of DNA with XhoI, at 37 &#176;C for 6 hr or O/N.</li>
	<li>Purify DNA by standard phenol:chloroform extraction and precipitate with ethanol. Resuspend in 20 &#956;l of deionized water (alternatively, commercial DNA fragment purification columns can be used).</li>
	<li>Run the undigested and digested DNA on a 1% agarose gel and determine the concentration of DNA by spectrometer reading. Alternatively, run samples at 1:1, 1:5, and 1:10 dilutions on a 1% agarose gel and quantify compared to a DNA ladder.</li>
	<li>Prepare an injection mix at a final concentration of 15 ng/&#956;l of digested rag2-kRASG12D DNA in 0.1 M KCl and 0.5x Tris-EDTA. The final DNA amount injected in 2 nl of injection volume will be 30 pg. 
	NOTE: Up to three different DNA constructs can be efficiently co-injected in a maximum of 60 pg of DNA per embryo. These transgenes become integrated into the genome and co-expressed within the developing tumor26.</li>
	<li>Inject linearized rag2-kRASG12D into one-cell stage embryos essentially as described27 into a zebrafish strain of interest (Figure 1B). Injections should be performed in the cell and not in the yolk for higher efficiency. In this experiment, a double transgenic AB-strain; myf5-GFP, mylpfa-mCherry was used. Raise zebrafish using standard rearing protocols28. 
	NOTE: Injection survival is often dependent upon the zebrafish strain used. On average, 30% of injected embryos will develop ERMS. 300-600 embryos should be injected per experiment in order to ensure that enough GFP-positive and mCherry-positive primary tumors are generated for transplantation and analysis.</li>
</ol>
5. Screening for Primary ERMS in Zebrafish Larvae
<ol>
	<li>Observe injected zebrafish from 10 to 30 days post injection for the emergence of externally visible primary ERMS.</li>
	<li>At 30 days post injection, anesthetize recipient zebrafish by adding single drops of tricaine methanesulfonate (MS222 4 mg/ml stock solution) into a Petri dish containing fish system water until operculum movements slow and fish are still. 
	NOTE: Dose of tricaine anesthesia will depend on the age and size of recipient zebrafish. Primary tumor-bearing zebrafish require lower doses of tricaine.</li>
	<li>Select primary ERMS-bearing fish that are myf5-GFP-positive and mylpfa-mCherry-positive, using an epifluorescence microscope.</li>
</ol>
6. ERMS Tumor Preparation
<ol>
	<li>Sacrifice selected primary ERMS-bearing zebrafish in 1.6 mg/ml tricaine methanesulfonate (MS222) for 10 min or until no operculum movement is evident.</li>
	<li>Process each tumor-bearing zebrafish separately. Place fish in a clean Petri dish and dissect around the tumor using a razor blade and fine forceps (as shown in Figure 1B). Transfer the dissected tumor tissue to a clean Petri dish.</li>
	<li>Add 100 &#956;l of pre-chilled 0.9x Phosphate Buffer Saline (PBS) supplemented with 5% Fetal Bovine Serum (FBS). Mince tissue with a clean razor blade &#62;20 times until cells are in a uniform suspension.</li>
	<li>Add 900 &#956;l of the same buffer (0.9x PBS + 5% FBS), pipette up and down several times to dissociate cells using a 1000 &#956;l filtered pipette tip. Filter through a 40 &#956;m mesh strainer into the corresponding 50 ml conical tube. Store on ice.</li>
	<li>Wash the Petri dish with an additional 2-4 ml of buffer, and pass through the same mesh strainer and into the corresponding conical tube.</li>
	<li>Centrifuge at 1,000 x g, for 10 min, at 4 &#176;C.</li>
	<li>Discard supernatant and resuspend in 100 &#956;l of buffer.</li>
	<li>Count the total number of viable cells using trypan blue dye and a hemocytometer.</li>
	<li>Dilute cells to desired concentration in the same buffer (0.9x PBS + 5% FBS). Cells should be diluted to 5 x 103 cells/&#956;l for transplanting 5 &#956;l per recipient zebrafish in a total of 2.5 x 104 cells per recipient.</li>
	<li>Flow Cytometry analysis can also be performed with a small amount of the suspension from step 6.5 to quantize the relative ratios of fluorescent cells within the sample. 
	NOTE: Set aside 100 &#956;l of cell suspension (following filtering in step 3.5) and dilute with 400 &#956;l of 0.9x PBS + 5% FBS suspension buffer for Flow Cytometry analysis. To ensure proper gating, perform additional analysis using single transgenic tumor tissue or muscle isolated from adult wild type, myf5-GFP and mylpfa-mCherry fish. Perform Flow Cytometry essentially as described in step 2 of Section 1.</li>
</ol>
7. Transplantation of ERMS into Adult rag2 Homozygous Mutant Zebrafish
<ol>
	<li>Clean a 10 &#956;l 26S G micro-syringe by drawing in and expelling 10% bleach solution (5 times), followed by 70% ethanol (5 times), and then followed by suspension buffer (0.9x PBS + 5% FBS, 10 times).</li>
	<li>Anesthetize recipient homozygous rag2 mutant fish by adding single drops of tricaine methanesulfonate (MS222 4 mg/ml stock solution) into a Petri dish containing the fish in system water until operculum movements are slow and fish are still.</li>
	<li>Place anesthetized recipient zebrafish on a wet paper towel or sponge, with the ventral side facing up.</li>
	<li>Inject 5 &#956;l of the cell suspension into the peritoneal cavity (2.5 x 104 cells per recipient). 
	NOTE: The injection needle should be cleaned between injections of different tumors as described in step 4.1. 5 to 10 &#956;l can be efficiently transplanted intraperitoneally, depending on recipient fish size. Tumor engraftment can be accomplished by injecting 1 x 104 to 5 x 105 unsorted cells per recipient fish (Table 1).</li>
	<li>Carefully place recipient zebrafish into a clean tank with a plastic spoon.</li>
	<li>Assess recipient zebrafish for engraftment rates at 10, 20, 30 days post-transplantation by imaging anesthetized fish under bright field and epifluorescence microscopy.</li>
	<li>Utilize engrafted fish for downstream applications including Fluorescence Activated Cell Sorting (FACS) to assess differentiation status (Figure 3H), standard histological analysis (Figure 3F), imaging therapy responses15, and/or serial transplantation approaches including limiting dilution analysis11.</li>
</ol>

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D. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=A+myogenic+precursor+cell+that+could+contribute+to+regeneration+in+zebrafish+and+its+similarity+to+the+satellite+cell.">A myogenic precursor cell that could contribute to regeneration in zebrafish and its similarity to the satellite cell.</a> The FEBS journal. 280 (17), 4074-4088 (2013).</li><li>Rowlerson, a., Radaelli, G., Mascarello, F., Veggetti, <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Regeneration+of+skeletal+muscle+in+two+teleost+fish:+Sparus+aurata+and+Brachydanio+rerio.">Regeneration of skeletal muscle in two teleost fish: Sparus aurata and Brachydanio rerio.</a> Cell Tissue Res. 289 (2), 311-322 (1997).</li><li>White, R. M., Sessa, A., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/entrez/query.fcgi?db=PubMed&cmd=Search&doptcmdl=Citation&defaultField=Title+Word&term=Transparent+adult+zebrafish+as+a+tool+for+in+vivo+transplantation+analysis.">Transparent adult zebrafish as a tool for in vivo transplantation analysis.</a> Cell stem cell. 2 (2), 183-189 (2008).</li></ol>

The authors have no competing financial interests.

Efficient and robust engraftment of adult dorsal skeletal muscle was attained with a very simple cell preparation method followed by injection of cells into the dorsal musculature of rag2 homozygous mutant fish. In general, intramuscular injection procedures were very robust, with some associated death immediately following the implantation procedure, ranging from 10% to 35% depending on experiment. Additional optimization will likely center on utilization of smaller gauge needles for injection and development of stationary injection apparatus using a microscope and micromanipulator, which will facilitate ease of implanting cells. Our approach also used unsorted muscle cells from donor animals and only contained approximately 30% muscle progenitor cells. Use of transgenic reporter lines that label stem cells and FACS isolation will likely provide enriched cell suspensions that lead to increased engraftment into recipient fish. Skeletal muscle cells could also be enriched and cultured prior to transplantation, as previously described29. Remarkably, our results also indicate that the steps of niche establishment and differentiation of donor muscle tissue occur before 10 days post transplantation, establishing this model as a robust and fast experimental platform to assess muscle engraftment and regeneration. Moreover, these experiments starkly contrast with those completed in mice, where pre-injury of muscle with cardiotoxin or barium chloride is required two days prior to engraftment30,31. It is likely that needle injury produced during the transplantation procedure potentiates engraftment by stimulating the production of a regenerative environment within the recipient animal32,33. We also envision that our method will be easily adapted to the transplantation of skeletal muscle tissue from younger zebrafish, allowing assessment of genetic mutations that affect early skeletal muscle development but lead to lethality at the larval stages.
We have also provided a detailed protocol for engraftment of zebrafish ERMS by intraperitoneal injection into non-conditioned, rag2 homozygous mutant fish. This approach was useful for expansion of double transgenic primary tumors without the need for generating tumors within a syngeneic transgenic line. Our recent work has shown that cell transplantation approaches provide novel experimental models to assess ERMS drug sensitivity in vivo, where a single tumor can be expanded into thousands of animals and assessed for effects on growth, self-renewal, and neovascularization15. Moreover, we have successfully engrafted a wide range of tumors into rag2 homozygous mutant fish including T cell acute lymphoblastic leukemia, melanoma, and ERMS23. Looking toward the future, we envision these lines will be useful for assessing important functional properties of cancer in vivo including assessing intra-tumoral heterogeneity, invasion, metastasis, angiogenesis, and therapy resistance. Moreover, the generation of rag2 homozygous mutant fish in the optically clear Casper strain zebrafish34 will likely facilitate direct imaging of many of these hallmarks of cancer.
In total, we provide detailed protocols for the successful engraftment of fluorescently-labeled normal and malignant skeletal muscle in to adult rag2 homozygous mutant immune compromised zebrafish.

Zebrafish are an excellent model for regenerative studies because they can regenerate amputated fins, as well as a damaged brain, retina, spinal cord, heart, skeletal muscle and other tissues1. Stem cell and regenerative studies in adult zebrafish have largely focused on the characterization of regeneration in response to injury, while identification of stem and progenitor cells from various tissues by cell transplantation has only recently been explored2. Zebrafish have also become increasingly used for the study of cancer through the generation of transgenic cancer models that mimic human disease3&#8211;10.
In the setting of cancer, cell transplantation approaches have become widely adopted and permit the dynamic assessment of important cancer processes including self-renewal11, functional heterogeneity12,13, neovascularization14, proliferation, therapy responses15, and invasion16,17. However, engrafted cells are often rejected from recipient fish due to host immune defenses that attack and kill the graft18. Several methods have been used to overcome rejection of engrafted cells. For example, the recipient animals immune system can be transiently ablated by low dose gamma-irradiation prior to transplantation18,19. However, the recipient immune system will recover by 20 days post-irradiation and kill donor cells18. Alternatively, dexamethasone treatment has been used to suppress T and B cell function, providing longer immune suppressive conditioning and facilitating engraftment of a wide range of human tumors for up to 30 days14. These experiments require constant drug dosing and are limited to study of solid tumors. Long-term engraftment assays have used genetically-identical syngeneic lines20&#8211;22, where the donor and recipient cells are immune matched. However, these models require transgenic lines of interest to be crossed into the syngeneic background for more than four generations to produce fully syngeneic lines. To obviate issues of immune rejection in recipient fish, our group has recently developed an immune compromised rag2E450fs homozygous mutant (ZFIN allele designation rag2fb101) line that have reduced T and B cell function and which permit engraftment of a wide range of tissues23. Similar immune compromised mouse models have been used extensively for cell transplantation of mouse and human tissues24.
Here, we present methods for transplantation of skeletal muscle and embryonal rhabdomyosarcoma (ERMS), a pediatric sarcoma that shares features with skeletal muscle, into the newly described rag2 homozygous mutant zebrafish. The availability of an immune compromised adult zebrafish expands our ability to perform large-scale cell transplantation studies to directly visualize and assess stem cell self-renewal within normal and malignant tissues. With this method, fluorescently labeled muscle cell preparations from adult &#945;-actin-RFP25 transgenic zebrafish robustly engraft in rag2 homozygous mutant zebrafish following injection into the dorsal musculature. Moreover, we demonstrate engraftment and expansion of primary myf5-GFP; mylpfa-mCherry transgenic ERMS following intraperitoneal injection into rag2E450fs homozygous mutant zebrafish. The utility of these protocols goes beyond the examples shown and can be easily applied to additional zebrafish regenerative tissues and cancers.

<table><tbody><tr><td>Tris-EDTA buffer solution 1x</td><td>Sigma-Aldrich</td><td>93283-100ML</td><td>Microinjection. Injection mix.</td></tr><tr><td>Potassium Chloride</td><td>Fisher Science Education</td><td>S77375-1</td><td>Microinjection. Injection mix.</td></tr><tr><td>XhoI Restriction Enzyme</td><td>New England Biolabs</td><td>R0146S</td><td>Microinjection. Plasmid linearization.</td></tr><tr><td>QIAquick PCR Purification Kit</td><td>Qiagen</td><td>28104 (50) or 28106 (250)</td><td>Microinjection. For purification of linearized plasmid up to 10 kb.</td></tr><tr><td>Phenol/Chloroform/Isoamyl Alcohol</td><td>Fisher Scientific</td><td>BP1753I-100</td><td>Microinjection. For purification of linearized plasmid.</td></tr><tr><td>UltraPure Agarose, 500&amp;nbsp;g</td><td>Invitrogen</td><td>16500-500</td><td>Microinjection. Linearized plasmid quantification.</td></tr><tr><td>Nanodrop 2000 Spectrophotometer</td><td>Thermo Scientific</td><td>http://www.nanodrop.com/Productnd2000overview.aspx</td><td>Microinjection. Linearized plasmid quantification.</td></tr><tr><td>DAPI (4&#039;,6-diamidino-2-phenylindole, dihydrochloride)</td><td>Life Technologies</td><td>D1306</td><td>flow cytometry/FACS</td></tr><tr><td>5 ml polystyrene round bottom tube</td><td>BD Falcon</td><td>352058</td><td>flow cytometry collection tube</td></tr><tr><td>BD FACSAria II</td><td>BD Biosciences</td><td>Special Order Research Products (SORP) program</td><td>FACS</td></tr><tr><td>5 ml polypropylene round bottom tube</td><td>BD Falcon</td><td>352063</td><td>FACS collection tube</td></tr><tr><td>BD LSR II</td><td>BD Biosciences</td><td>Special Order Research Products (SORP) program</td><td>flow cytometry</td></tr><tr><td>Phosphate Buffered Saline, pH 7.4 (1x)</td><td>Life Technologies</td><td>10010-023</td><td>transplantation</td></tr><tr><td>Fetal Bovine Serum</td><td>Omega Scientific</td><td>FB-01</td><td>transplantation</td></tr><tr><td>Tricaine methanesulphonate (MS-222)</td><td>Western Chemical Inc.</td><td>http://www.wchemical.com/tricaine-s-ms-222.html</td><td>Transplantation. Anesthetic. Caution: Irritant. Irritating to eyes, respiratory system, and skin.</td></tr><tr><td>VWR Absorbent Bench Underpads</td><td>VWR</td><td>56616-018</td><td>Transplantation. Regular paper towels or sponge can be used as an alternative.</td></tr><tr><td>Singe Edge Industrial Razor Blades</td><td>VWR</td><td>55411-050</td><td>transplantation</td></tr><tr><td>Petri Dish, Polystryrene Disposable Sterile</td><td>VWR</td><td>25384-302</td><td>transplantation</td></tr><tr><td>Cell Strainer, 40 &amp;micro;m Nylon</td><td>Falcon-Corning Incorporated</td><td>352340</td><td>transplantation</td></tr><tr><td>50 ml Centrifuge Tube</td><td>Corning Incorporated</td><td>430828</td><td>transplantation</td></tr><tr><td>Trypan Blue Stain (0.4%)</td><td>Life Technologies</td><td>15250-061</td><td>transplantation</td></tr><tr><td>Hemacytometer Set&amp;nbsp;</td><td>Hausser Scientific</td><td>1483</td><td>transplantation</td></tr><tr><td>Hamilton syringe, fixed needle, volume 10 &amp;micro;l, needle size 26s ga (bevel tip)</td><td>Hamilton</td><td>80366</td><td>transplantation</td></tr><tr><td>Austin&#039;s A-1 Bleach, Commercial</td><td>James Austin Company</td><td></td><td>Transplantation. Any commercial solution can be used.</td></tr><tr><td>Ethanol 190 Proof</td><td>Decon Labs, Inc.</td><td>DSP-MD.43</td><td>Microinjection (linearized plasmid purification) and transplantation. Any commercial&amp;nbsp; solution can be used.</td></tr><tr><td>High Speed Microcentrifuge, 300D Digital Microcentrifuge</td><td>Denville Scientific Inc.</td><td>C0265-24</td><td>transplantation</td></tr><tr><td>Sorvall Legend XFR Centrifuge</td><td>Thermo Scientific</td><td>75004539&amp;nbsp;</td><td>Transplantation. Catalog number for 120 V, 60 Hz (US).</td></tr><tr><td>5 ml serological pipets</td><td>BD Falcon</td><td>357529</td><td>transplantation</td></tr><tr><td>Corning Stripettor Plus Pipetting Controller</td><td>Corning Incorporated</td><td>4090</td><td>Transplantation. Any automatic pipetting controller can be used.</td></tr><tr><td>Powder free examination gloves</td><td></td><td></td><td>All steps. Any commercial brand can be used.</td></tr><tr><td>Filter pipet tips and micropipettes</td><td></td><td></td><td>All steps. Any commercial brand can be used.</td></tr><tr><td>Dumont forceps #5</td><td>Fine Science Tools</td><td>11205-20</td><td>transplantation</td></tr><tr><td>Fluorescent Stereomicroscope</td><td>Olympus</td><td>MVX10</td><td>Scoring. Any appropriate fluorescent stereomicroscope can be used.</td></tr><tr><td>Olympus DP72 microscope digital camera</td><td>Olympus</td><td>DP72</td><td>Scoring. Multiple adequate cameras for the selected imaging system can be used.</td></tr></tbody></table>

normal and malignant muscle cell transplantation into immune compromised adult zebrafish

Zebrafish have become a powerful tool for assessing development, regeneration, and cancer. More recently, allograft cell transplantation protocols have been developed that permit engraftment of normal and malignant cells into irradiated, syngeneic, and immune compromised adult zebrafish. These models when coupled with optimized cell transplantation protocols allow for the rapid assessment of stem cell function, regeneration following injury, and cancer. Here, we present a method for cell transplantation of zebrafish adult skeletal muscle and embryonal rhabdomyosarcoma (ERMS), a pediatric sarcoma that shares features with embryonic muscle, into immune compromised adult rag2E450fs homozygous mutant zebrafish. Importantly, these animals lack T cells and have reduced B cell function, facilitating engraftment of a wide range of tissues from unrelated donor animals. Our optimized protocols show that fluorescently labeled muscle cell preparations from &#945;-actin-RFP transgenic zebrafish engraft robustly when implanted into the dorsal musculature of rag2 homozygous mutant fish. We also demonstrate engraftment of fluorescent-transgenic ERMS where fluorescence is confined to cells based on differentiation status. Specifically, ERMS were created in AB-strain myf5-GFP; mylpfa-mCherry double transgenic animals and tumors injected into the peritoneum of adult immune compromised fish. The utility of these protocols extends to engraftment of a wide range of normal and malignant donor cells that can be implanted into dorsal musculature or peritoneum of adult zebrafish.

A procedure for preparing and transplanting skeletal muscle cells from &#945;-actin-RFP transgenic donors into immune compromised homozygous rag2 mutant zebrafish has been demonstrated (Protocol Section 1, Figure 1A and Figure 2). Skeletal muscle tissue was prepared from &#945;-actin-RFP transgenic donors and the resulting single cell suspension contained 84.3% viable cells as assessed by DAPI exclusion following Flow Cytometry analysis (Figure 2B). RFP-positive cells comprised 35.3% of this single cell suspension (Figure 2C). Transplantation of cells into the dorsal skeletal muscle of rag2 homozygous mutant recipient fish led to consistent and strong engraftment as assessed by differentiation of single cells into multinucleated fibers (1 x 106 cells injected per fish, Table 1, Figure 2D-I). Wild type recipient fish failed to engraft muscle fibers over the 30-day experiment (n = 13). By 10 days post transplantation, 9 out of 14 rag2 homozygous mutant zebrafish contained RFP-positive muscle fibers near the site of injection (64.3%, Figure 2E,F). Importantly, engrafted RFP-positive muscle persisted to 30 days post-transplantation (Figure 2G-I), with a subset of animals being followed for 115 days post-engraftment and exhibiting robust and persistent muscle engraftment (data not shown). These results are similar to those reported previously by our group23 using the same protocol (Table 1).
We have also presented a method for the generation, preparation and transplantation of ERMS tumor cells into the peritoneal cavity of rag2 homozygous mutant recipient fish (Protocol Section 2, Figure 1B and Figure 3). ERMS were generated in double transgenic myf5-GFP; mylpfa-mCherry fish that have been shown to allow the visualization of intra-tumoral heterogeneity and functional analysis of tumor cell subpopulations following transplantation11. However, further molecular characterization of each subpopulation is difficult because fish are small when they develop ERMS between 10 to 30 days of life and the number of tumor cells are limiting for downstream applications. One solution is to expand tumor cell numbers by engrafting ERMS into adult recipient zebrafish. To date, similar experiments have been completed using CG1-strain syngeneic fish and required in excess of 4 generations of backcrossing to develop syngeneic lines that were transgenic for myf5-GFP; mylpfa-mCherry. To circumvent these issues, we demonstrated the utility of immune compromised rag2 homozygous mutant recipient zebrafish to engraft primary ERMS from a AB-strain zebrafish. All primary ERMS engrafted into rag2 homozygous mutant animals, facilitating expansion of the tumor (Table 1). Similar results were recently reported where 24 of 27 rag2 homozygous mutant zebrafish engrafted ERMS, while 0 of 7 wild type siblings engrafted disease23. A representative example of an engrafted ERMS is shown at 30 days post-transplantation in Figure 3E. Engrafted ERMS share histological features of embryonal rhabdomyosarcoma, similar to that found in the primary tumor (Figure 3B and 3F). FACS analysis confirmed that ERMS contained functionally distinct tumor propagating cells and differentiated cells that express myf5-GFP and/or mylpfa-mCherry. Survival rates following the intraperitoneal injection procedure were in excess of 95%. Recipient zebrafish commonly succumb from tumor burden after the 30 days post-transplantation time point.
<img alt="Figure 1" src="/files/ftp_upload/52597/52597fig1highres.jpg" width="700px" /> 
Figure 1. Protocol schematic for (A) normal and (B) malignant skeletal muscle cell transplantation into rag2 homozygous mutant zebrafish. Optional steps are marked with (*).
<img alt="Figure 2" src="/files/ftp_upload/52597/52597fig2highres.jpg" width="700px" /> 
Figure 2. Skeletal muscle engraftment into rag2 homozygous mutant zebrafish. (A) &#945;-actin-RFP transgenic donor zebrafish. (B) Cell viability of isolated muscle cell suspension as assessed by DAPI dye exclusion and flow cytometry. (C) Proportion of RFP-positive cells found within the muscle cell suspension from &#945;-actin-RFP donor (red), compared to a wild type control (grey). (D-E) Merged bright field and fluorescent images of wild type animals (D) or rag2 homozygous mutant fish (E) at 30 days post-transplantation. (F) Engraftment rates over time. Red denotes number of engrafted animals while grey shows non-engrafted fish. Number of animals analyzed at each time point are indicated. (G-I) High magnification images of boxed region in panel E shown at 10 (G), 20 (H) and 30 (I) days post-transplantation, showing retention of differentiated muscle fibers over time (arrowheads). Scale bars equal 2 mm. <a href="https://www.jove.com/files/ftp_upload/52597/52597fig2highres.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" src="/files/ftp_upload/52597/52597fig3highres.jpg" width="700px" /> 
Figure 3. Transplantation of myf5-GFP; mylpfa-mCherry ERMS into rag2 homozygous mutant zebrafish. (A-D) rag2-kRASG12D induced primary ERMS arising in AB-strain myf5-GFP; mylpfa-mCherry zebrafish at 30 days of life. (E-H) rag2 homozygous mutant zebrafish engrafted with ERMS and analyzed at 30 days post-transplantation. (A, E) Merged bright field and fluorescent images of primary and transplanted ERMS. Tumor area is outlined and arrowhead indicates injection site in E. (B, F) Hematoxylin- and eosin-stained paraffin sections of primary (B) and engrafted ERMS (F) showing areas of increased cellularity associated with cancer. (C, G) Cell viability as assessed by DAPI dye exclusion and flow cytometry. (D, H) Fluorescent tumor cell sub-populations, as assessed by flow cytometry. Scale bars equal 2 mm (A, E) and 50 &#956;m (B, F). <a href="https://www.jove.com/files/ftp_upload/52597/52597fig3highres.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Table 1" src="/files/ftp_upload/52597/52597table1.jpg" width="700px" /> 
Table 1. Engraftment results for muscle and ERMS cell transplantation. (*) denotes previously reported data using the same techniques23. Data is reprinted with permission from Nature Methods. <a href="https://www.jove.com/files/ftp_upload/52597/52597table1.jpg" target="_blank">Please click here to view a larger version of this table.</a>

Watch this Scientific Journal Video about Normal and Malignant Muscle Cell Transplantation into Immune Compromised Adult Zebrafish at JoVE.com

Normal and Malignant Muscle Cell Transplantation into Immune Compromised Adult Zebrafish

Here, we present a protocol for cell transplantation of zebrafish skeletal muscle and embryonal rhabdomyosarcoma (ERMS) into adult immune compromised rag2E450fs homozygous mutant zebrafish. This protocol allows for the efficient analysis of regeneration and malignant transformation of muscle cells.

Zebrafish have become a powerful tool for assessing development, regeneration, and cancer. More recently, allograft cell transplantation protocols have ...

normal-malignant-muscle-cell-transplantation-into-immune-compromised

Nanyang Technological University

Research

JoVE Journal

Immunology and Infection

10.9K Views.  Massachusetts General Hospital. Here, we present a protocol for cell transplantation of zebrafish skeletal muscle and embryonal rhabdomyosarcoma (ERMS) into adult immune compromised rag2E450fs homozygous mutant zebrafish. This protocol allows for the efficient analysis of regeneration and malignant transformation of muscle cells. 

Video: Normal and Malignant Muscle Cell Transplantation into Immune Compromised Adult Zebrafish

Transplantation of Whole Kidney Marrow in Adult Zebrafish

Hematopoietic stem cells (HSC) are a rare population of pluripotent cells that maintain all the differentiated blood lineages throughout the life of an organism. The functional definition of a HSC is a transplanted cell that has the ability to reconstitute all the blood lineages of an irradiated recipient long term. This designation was established by decades of seminal work in mammalian systems. Using hematopoietic cell transplantation (HCT) and reverse genetic manipulations in the mouse, the underlying regulatory factors of HSC biology are beginning to be unveiled, but are still largely under-explored. Recently, the zebrafish has emerged as a powerful genetic model to study vertebrate hematopoiesis. Establishing HCT in zebrafish will allow scientists to utilize the large-scale genetic and chemical screening methodologies available in zebrafish to reveal novel mechanisms underlying HSC regulation. In this article, we demonstrate a method to perform HCT in adult zebrafish. We show the dissection and preparation of zebrafish whole kidney marrow, the site of adult hematopoiesis in the zebrafish, and the introduction of these donor cells into the circulation of irradiated recipient fish via intracardiac injection. Additionally, we describe the post-transplant care of fish in an "ICU" to increase their long-term health. In general, gentle care of the fish before, during, and after the transplant is critical to increase the number of fish that will survive more than one month following the procedure, which is essential for assessment of long term (&lt;3 month) engraftment. The experimental data used to establish this protocol will be published elsewhere. The establishment of this protocol will allow for the merger of large-scale zebrafish genetics and transplant biology.

In this article, we demonstrate a method to perform HCT in adult zebrafish.

Hematopoietic stem cells (HSC) are a rare population of pluripotent cells that maintain all the differentiated blood lineages throughout the life of an ...

Biology

Transplantation of Zebrafish Pediatric Brain Tumors into Immune-competent Hosts for Long-term Study of Tumor Cell Behavior and Drug Response

Tumor cell transplantation is an important technique to define the mechanisms controlling cancer cell growth, migration, and host response, as well as to assess potential patient response to therapy. Current methods largely depend on using syngeneic or immune-compromised animals to avoid rejection of the tumor graft. Such methods require the use of specific genetic strains that often prevent the analysis of immune-tumor cell interactions and/or are limited to specific genetic backgrounds. An alternative method in zebrafish takes advantage of an incompletely developed immune system in the embryonic brain before 3 days, where tumor cells are transplanted for use in short-term assays (i.e., 3 to 10 days). However, these methods cause host lethality, which prevents the long-term study of tumor cell behavior and drug response. This protocol describes a simple and efficient method for the long-term orthotopic transplantation of zebrafish brain tumor tissue into the fourth ventricle of a 2-day-old immune-competent zebrafish. This method allows: 1) long-term study of tumor cell behaviors, such as invasion and dissemination; 2) durable tumor response to drugs; and 3) re-transplantation of tumors for the study of tumor evolution and/or the impact of different host genetic backgrounds. In summary, this technique allows cancer researchers to assess engraftment, invasion, and growth at distant sites, as well as to perform chemical screens and cell competition assays over many months. This protocol can be extended to studies of other tumor types and can be used to elucidate mechanisms of chemoresistance and metastasis.

The transplantation of cancer cells is an important tool for the identification of cancer mechanisms and therapeutic responses. Current techniques depend on immune-incompetent animals. Here, we describe a method to transplant zebrafish tumor cells into immune-competent embryos for the long-term analysis of tumor cell behavior and in vivo drug responses.

Tumor cell transplantation is an important technique to define the mechanisms controlling cancer cell growth, migration, and host response, as well as to ...

Cancer Research

Tissue Targeted Embryonic Chimeras: Zebrafish Gastrula Cell Transplantation

Certain fundamental questions in the field of developmental biology can only be answered when cells are placed in novel environments or when small groups of cells in a larger context are altered.  Watching how one cell interacts with and behaves in a unique environment is essential to characterizing cell functions.  Determining how the localized misexpression of a specific protein influences surrounding cells provides insightful information on the roles that protein plays in a variety of developmental processes.  Our lab uses the zebrafish model system to uniquely combine genetic approaches with classical transplantation techniques to generate genotypic or phenotypic chimeras.  We study neuron-glial cell interactions during the formation of forebrain commissures in zebrafish. This video describes a method that allows our lab to investigate the role of astroglial populations in the diencephalon and the roles of specific guidance cues that influence projecting axons as they cross the midline. Due to their transparency zebrafish embryos are ideal models for this type of ectopic cell placement or localized gene misexpression. Tracking transplanted cells can be accomplished using a vital dye or a transgenic fish line expressing a fluorescent protein. We demonstrate here how to prepare donor embryos with a vital dye tracer for transplantation, as well as how to extract and transplant cells from one gastrula staged embryo to another.  We present data showing ectopic GFP+ transgenic cells within the forebrain of zebrafish embryos and characterize the location of these cells with respect to forebrain commissures.  In addition, we show laser scanning confocal timelapse microscopy of Alexa 594 labeled cells transplanted into a GFP+ transgenic host embryo.  These data provide evidence that gastrula staged transplantation enables the targeted positioning of ectopic cells to address a variety of questions in Developmental Biology.

Zebrafish cell transplantation enables the combination of genetics and embryology to generate tissue specific chimeras. This video demonstrates gastrula staged cell transplantations that have allowed our lab to investigate the roles of astroglial populations and specific guidance cues during commissure formation in the forebrain.

Certain fundamental questions in the field of developmental biology can only be answered when cells are placed in novel environments or when small groups ...

Examining Muscle Regeneration in Zebrafish Models of Muscle Disease

Skeletal muscle has a remarkable ability to regenerate following injury, which is driven by obligate tissue resident muscle stem cells. Following injury, the muscle stem cell is activated and undergoes cell proliferation to generate a pool of myoblasts, which subsequently differentiate to form new muscle fibers. In many muscle wasting conditions, including muscular dystrophy and ageing, this process is impaired resulting in the inability of muscle to regenerate. The process of muscle regeneration in zebrafish is highly conserved with mammalian systems providing an excellent system to study muscle stem cell function and regeneration, in muscle wasting conditions such as muscular dystrophy. Here, we present a method to examine muscle regeneration in zebrafish models of muscle disease. The first step involves the use of a genotyping platform that allows the determination of the genotype of the larvae prior to eliciting an injury. Having determined the genotype, the muscle is injured using a needle stab, following which polarizing light microscopy is used to determine the extent of muscle regeneration. We therefore provide a high throughput pipeline which allows the examination of muscle regeneration in zebrafish models of muscle disease.

Skeletal muscle regeneration is driven by tissue resident muscle stem cells, which are impaired in many muscle diseases such as muscular dystrophy, and this results in the inability of muscle to regenerate. Here, we describe a protocol that allows the examination of muscle regeneration in zebrafish models of muscle disease.

Skeletal muscle has a remarkable ability to regenerate following injury, which is driven by obligate tissue resident muscle stem cells. Following injury, ...

Developmental Biology

Estimating LSC Frequency in Zebrafish T-ALL Using Cell Proliferation Dye Sorting

Identification of Quiescent Cells in a Zebrafish T-Cell Acute Lymphoblastic Leukemia Model Using Cell Proliferation Staining

Cellular quiescence is a state of growth arrest or slowed proliferation that is described in normal and cancer stem cells (CSCs). Quiescence may protect CSCs from antiproliferative chemotherapy drugs. In T-cell acute lymphoblastic leukemia (T-ALL) patient-derived xenograft (PDX) mouse models, quiescent cells are associated with treatment resistance and stemness. Cell proliferation dyes are popular tools for the tracking of cell division. The fluorescent dye is covalently anchored into amine groups on the membrane and macromolecules inside the cell. This allows for the tracking of labeled cells for up to 10 divisions, which can be resolved by flow cytometry.
Ultimately, cells with the highest proliferation rates will have low dye retention, as it will be diluted with each cell division, while dormant, slower-dividing cells will have the highest retention. The use of cell proliferation dyes to isolate dormant cells has been optimized and described in T-ALL mouse models. Complementary to the existing mouse models, the rag2:Myc-derived zebrafish T-ALL model provides an excellent venue to interrogate self-renewal in T-ALL due to the high frequency of leukemic stem cells (LSCs) and the convenience of zebrafish for large-scale transplant experiments.
Here, we describe the workflow for the staining of zebrafish T-ALL cells with a cell proliferation dye, optimizing the concentration of the dye for zebrafish cells, passaging successfully stained cells in vivo, and the collection of cells with varying levels of dye retention by live cell sorting from transplanted animals. Given the absence of well-established cell surface makers for LSCs in T-ALL, this approach provides a functional means to interrogate quiescent cells in vivo. For representative results, we describe the engraftment efficiency and the LSC frequency of high and low dye-retaining cells. This method can help investigate additional properties of quiescent cells, including drug response, transcriptional profiles, and morphology.

Author Spotlight: Identification and Isolation of Quiescent Leukemia Stem Cells from Zebrafish T-ALL

We used cell proliferation staining to identify quiescent cells in the zebrafish T-acute lymphoblastic leukemia model. The stain is retained in non-dividing cells and reduced during cell proliferation, enabling the selection of dormant cells for further interrogation. This protocol provides a functional tool to study self-renewal in the context of cellular quiescence.

Cellular quiescence is a state of growth arrest or slowed proliferation that is described in normal and cancer stem cells (CSCs). Quiescence may protect ...

Utilizing Larval Zebrafish for Efficient In Vivo Tumor Studies

A Simple, Rapid, and Effective Method for Tumor Xenotransplantation Analysis in Transparent Zebrafish Embryos

In vivo studies of tumor behavior are a staple of cancer research; however, the use of mice presents significant challenges in cost and time. Here, we present larval zebrafish as a transplant model that has numerous advantages over murine models, including ease of handling, low expense, and short experimental duration. Moreover, the absence of an adaptive immune system during larval stages obviates the need to generate and use immunodeficient strains. While established protocols for xenotransplantation in zebrafish embryos exist, we present here an improved method involving embryo staging for faster transfer, survival analysis, and the use of flow cytometry to assess disease burden. Embryos are staged to facilitate rapid cell injection into the yolk of the larvae and cell marking to monitor the consistency of the injected cell bolus. After injection, embryo survival analysis is assessed up to 7 days post injection (dpi). Finally, disease burden is also assessed by marking transferred cells with a fluorescent protein and analysis by flow cytometry. Flow cytometry is enabled by a standardized method of preparing cell suspensions from zebrafish embryos, which could also be used in establishing the primary culture of zebrafish cells. In summary, the procedure described here allows a more rapid assessment of the behavior of tumor cells in vivo with larger numbers of animals per study arm and in a more cost-effective manner.

Author Spotlight: Advancing Cancer Therapeutics Using Tumor Xenotransplantation in Zebrafish

We describe a protocol for xenotransplantation into the yolk of transparent zebrafish embryos that is optimized by a simple, rapid staging method. Post-injection analyses include survival and assessing the disease burden of xenotransplanted cells by flow cytometry.

In vivo studies of tumor behavior are a staple of cancer research; however, the use of mice presents significant challenges in cost and time. Here, we ...

A Simple and Effective Transplantation Device for Zebrafish Embryos

Classical embryological manipulations, such as removing cells and transplanting cells within or between embryos, are powerful techniques to study complex developmental processes. Zebrafish embryos are ideally suited for these manipulations since they are easily accessible, relatively large in size, and transparent. However, previously developed devices for cell removal and transplantation are cumbersome to use or expensive to purchase. In contrast, the transplantation device presented here is economical, easy to assemble, and simple to use. In this protocol, we first introduce the handling of the transplantation device as well as its assembly from commercially and widely available parts. We then present three applications for its use: generation of ectopic clones to study signal dispersal from localized sources, extirpation of cells to produce size-reduced embryos, and germline transplantation to generate maternal-zygotic mutants. Finally, we show that the tool can also be used for embryological manipulations in other species such as the Japanese rice fish medaka.

Embryological manipulations such as extirpation and transplantation of cells are important tools to study early development. This protocol describes a simple and effective transplantation device to perform these manipulations in zebrafish embryos.

Classical embryological manipulations, such as removing cells and transplanting cells within or between embryos, are powerful techniques to study complex ...

Transplantation of Cells Directly into the Kidney of Adult Zebrafish

Regenerative medicine based on the transplantation of stem or progenitor cells into damaged tissues has the potential to treat a wide range of chronic diseases1. However, most organs are not easily accessible, necessitating the need to develop surgical methods to gain access to these structures. In this video article, we describe a method for transplanting cells directly into the kidney of adult zebrafish, a popular model to study regeneration and disease2. Recipient fish are pre-conditioned by irradiation to suppress the immune rejection of the injected cells3. We demonstrate how the head kidney can be exposed by a lateral incision in the flank of the fish, followed by the injection of cells directly in to the organ. Using fluorescently labeled whole kidney marrow cells comprising a mixed population of renal and hematopoietic precursors, we show that nephron progenitors can engraft and differentiate into new renal tissue - the gold standard of any cell-based regenerative therapy. This technique can be adapted to deliver purified stem or progenitor cells and/or small molecules to the kidney as well as other internal organs and further enhances the zebrafish as a versatile model to study regenerative medicine.

Cell transplantation is an essential technique for studying tissue regeneration and for developing cell-based therapies of disease. We demonstrate here a microsurgical technique that permits the transplantation of genetically labeled cells directly into the kidney of adult zebrafish fish.

Regenerative medicine based on the transplantation of stem or progenitor cells into damaged tissues has the potential to treat a wide range of chronic ...

Robust Zebrafish Cell Transplantation for Regeneration and Development Research

High-resolution Cell Transplantation in Embryonic and Larval Zebrafish

Development and regeneration occur by a process of genetically encoded spatiotemporally dynamic cellular interactions. The use of cell transplantation between animals to track cell fate and to induce mismatches in the genetic, spatial, or temporal properties of donor and host cells is a powerful means of examining the nature of these interactions. Organisms such as chick and amphibians have made crucial contributions to our understanding of development and regeneration, respectively, in large part because of their amenability to transplantation. The power of these models, however, has been limited by low genetic tractability. Likewise, the major genetic model organisms have lower amenability to transplantation. 
The zebrafish is a major genetic model for development and regeneration, and while cell transplantation is common in zebrafish, it is generally limited to the transfer of undifferentiated cells at the early blastula and gastrula stages of development. In this article, we present a simple and robust method that extends the zebrafish transplantation window to any embryonic or larval stage between at least 1 and 7 days post fertilization. The precision of this approach allows for the transplantation of as little as one cell with near-perfect spatial and temporal resolution in both donor and host animals. While we highlight here the transplantation of embryonic and larval neurons for the study of nerve development and regeneration, respectively, this approach is applicable to a wide range of progenitor and differentiated cell types and research questions.

Author Spotlight: Mapping Cellular Connectivity in the Zebrafish Nervous System During Development and Regeneration

Here we present a protocol to transplant cells with high spatial and temporal resolution in zebrafish embryos and larvae at any stage between at least 1 and 7 days post fertilization.

Development and regeneration occur by a process of genetically encoded spatiotemporally dynamic cellular interactions. The use of cell transplantation ...

Isolating Malignant and Non-Malignant B Cells from lck:eGFP Zebrafish

Zebrafish (Danio rerio) are a powerful model to study lymphocyte development. Like mammals, D. rerio possess an adaptive immune system that includes B and T lymphocytes. Studies of zebrafish lymphopoiesis are difficult because antibodies recognizing D. rerio cell surface markers are generally not available, complicating isolation and characterization of different lymphocyte populations, including B-lineage cells. Transgenic lines with lineage-specific fluorophore expression are often used to circumvent this challenge. The transgenic lck:eGFP line has been used to study D. rerio T cell development, and has also been utilized to model T cell development and acute lymphoblastic leukemia (T-ALL). Although lck:eGFP fish have been widely used to analyze the T-lineage, they have not been used to study B cells. Recently, we discovered that many zebrafish B cells also express lck, albeit at lower levels. Consequently, lck:eGFP B cells likewise express low levels of GFP. Based on this finding, we developed a protocol to purify B-lineage cells from lck:eGFP zebrafish, which we report here. Our method describes how to utilize a fluorescent-activated cell sorter (FACS) to purify B cells from lck:eGFP fish or related lines, such as double-transgenic rag2:hMYC; lck:eGFP fish. In these lines, B cells, particularly immature B cells, express GFP at low but detectable levels, allowing them to be distinguished from T cells, which express GFP highly. B cells can be isolated from marrow, thymus, spleen, blood, or other tissues. This protocol provides a new method to purify D. rerio B cells, enabling studies focused on topics like B cell development and B lymphocyte malignancies.

Isolating Malignant and Non-Malignant B Cells from lck:eGFP Zebrafish

Transgenic lck:eGFP zebrafish express GFP highly in T lymphocytes, and have been used to study T cell development and acute lymphoblastic leukemia. This line can be used to study B cells, which express lck at lower levels. This protocol describes purification of malignant and non-malignant B cells from lck:eGFP zebrafish.

Zebrafish (Danio rerio) are a powerful model to study lymphocyte development. Like mammals, D. rerio possess an adaptive immune system that includes B and ...

Normal and Malignant Muscle Cell Transplantation into Immune Compromised Adult Zebrafish

Summary

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Chapters in this video

Transplantation of Whole Kidney Marrow in Adult Zebrafish

Transplantation of Zebrafish Pediatric Brain Tumors into Immune-competent Hosts for Long-term Study of Tumor Cell Behavior and Drug Response

Tissue Targeted Embryonic Chimeras: Zebrafish Gastrula Cell Transplantation

Examining Muscle Regeneration in Zebrafish Models of Muscle Disease

Identification of Quiescent Cells in a Zebrafish T-Cell Acute Lymphoblastic Leukemia Model Using Cell Proliferation Staining

A Simple, Rapid, and Effective Method for Tumor Xenotransplantation Analysis in Transparent Zebrafish Embryos

A Simple and Effective Transplantation Device for Zebrafish Embryos

Transplantation of Cells Directly into the Kidney of Adult Zebrafish

High-resolution Cell Transplantation in Embryonic and Larval Zebrafish

Isolating Malignant and Non-Malignant B Cells from lck:eGFP Zebrafish