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 border="0" cellpadding="0" cellspacing="0" width="1077">
	<tbody>
		<tr>
			<td>Name of Material/ Equipment</td>
			<td>Company</td>
			<td>Catalog Number</td>
			<td>Comments/Description</td>
		</tr>
		<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 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&#39;,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>Transportation</td>
		</tr>
		<tr>
			<td>Fetal Bovine Serum</td>
			<td>Omega Scientific</td>
			<td>FB-01</td>
			<td>Transportation</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>Transportation. 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>Transportation. 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>Transportation</td>
		</tr>
		<tr>
			<td>Petri Dish, Polystryrene Disposable Sterile</td>
			<td>VWR</td>
			<td>25384-302</td>
			<td>Transportation</td>
		</tr>
		<tr>
			<td>Cell Strainer, 40 &#181;m Nylon</td>
			<td>Falcon-Corning Incorporated</td>
			<td>352340</td>
			<td>Transportation</td>
		</tr>
		<tr>
			<td>50 mL Centrifuge Tube</td>
			<td>Corning Incorporated</td>
			<td>430828</td>
			<td>Transportation</td>
		</tr>
		<tr>
			<td>Trypan Blue Stain (0.4%)</td>
			<td>Life Technologies</td>
			<td>15250-061</td>
			<td>Transportation</td>
		</tr>
		<tr>
			<td>Hemacytometer Set&#160;</td>
			<td>Hausser Scientific</td>
			<td>1483</td>
			<td>Transportation</td>
		</tr>
		<tr>
			<td>Hamilton syringe, fixed needle, volume 10 &#181;L, needle size 26s ga (bevel tip)</td>
			<td>Hamilton</td>
			<td>80366</td>
			<td>Transportation</td>
		</tr>
		<tr>
			<td>Austin&#39;s A-1 Bleach, Commercial</td>
			<td>James Austin Company</td>
			<td></td>
			<td>Transportation. Any commercial&#160; 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 Transportation. Any commercial&#160; 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>Transportation</td>
		</tr>
		<tr>
			<td>Sorvall Legend XFR Centrifuge</td>
			<td>Thermo Scientific</td>
			<td>75004539&#160;</td>
			<td>Transportation. Catalog number for 120V, 60Hz (US)</td>
		</tr>
		<tr>
			<td>5 ml serological pipets</td>
			<td>BD Falcon</td>
			<td>357529</td>
			<td>Transportation</td>
		</tr>
		<tr>
			<td>Corning Stripettor Plus Pipetting Controller</td>
			<td>Corning Incorporated</td>
			<td>4090</td>
			<td>Transportation. 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>Transportation</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

Research

JoVE Journal

Immunology and Infection

10.8K 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

Flow Cytometry Analysis of Immune Cells Within Murine Aortas

Atherosclerosis is a chronic inflammatory process of medium and large size vessels that is characterized by the formation of plaques consisting of foam cells, immune cells, vascular endothelial and smooth muscle cells, platelets, extracellular matrix, and a lipid-rich core with extensive necrosis and fibrosis of surrounding tissues.1 The innate and adaptive arms of the immune response are involved in the initiation, development and persistence of atherosclerosis.2, 3 There is a significant body of evidence that different subsets of the immune cells, such as macrophages, dendritic cells, T and B lymphocytes, are present within the aortas of healthy and atherosclerosis-prone mice4. Additionally, immune cells are found in the surrounding aortic adventitia which suggests an important role of this tissue in atherogenesis.2
For some time, the quantitative detection of different types of immune cells, their activation status, and the cellular composition within the aortic wall was limited by RT-PCR and immunohistochemical methods for the study of atherosclerosis. Few attempts were made to perform flow cytometry using human aortas, and a number of problems, such as a high autofluorescence, have been reported5,6. Human atherosclerotic plaques were digested with collagenase 1, and free cells were collected and stained for CD14+/CD11c+ to highlight macrophage-derived foam cells. In this study, a "mock" channel was used to avoid false-positive staining.6 Necrotic materials accumulating during the digestion process give rise in a large amount of debris that generates a high autofluorescence in aortic samples. To resolve this problem, a panel of negative and positive controls has been proposed, but only double staining could be applied in these samples. We have developed a new flow cytometry-based method7 to analyze the immune cell composition and characterize the activation, proliferation, differentiation of immune cells in healthy and atherosclerosis-prone aorta. This method allows the investigation of the immune cell composition of the aortic wall and opens possibilities to use a broad spectrum of immunological methods for investigations of immune aspects of this disease.

This paper presents a flow cytometry-based method to investigate the immune composition of aortas. The paper also illustrates an additional technique that allows examining surrounding adventitia and vessel wall separately. This method opens possibilities to perform phenotypical analyses of aortic leukocytes and apply several immunological assays for atherosclerosis studies.

Atherosclerosis is a chronic inflammatory process of medium and large size vessels that is characterized by the formation of plaques consisting of foam ...

Isolation of Functional Cardiac Immune Cells

Cardiac immune cells are gaining interest for the roles they play in the pathological remodeling in many cardiac diseases.1-5 These immune cells, which include mast cells, T-cells and macrophages; store and release a variety of biologically active mediators including cytokines and proteases such as tryptase.6-8 These mediators have been shown to be key players in extracellular matrix metabolism by activating matrix metalloproteinases or causing collagen accumulation by modulating the cardiac fibroblasts' function.9-11 However, available techniques for isolating cardiac immune cells have been problematic because they use bacterial collagenase to digest the myocardial tissue. This technique causes activation of the immune cells and thus a loss of function. For example, cardiac mast cells become significantly less responsive to compounds that cause degranulation.12 Therefore, we developed a technique that allows for the isolation of functional cardiac immune cells which would lead to a better understanding of the role of these cells in cardiac disease.13, 14
This method requires a familiarity with the anatomical location of the rat's xiphoid process, axilla and falciform ligament, and pericardium of the heart. These landmarks are important to increase success of the procedure and to ensure a higher yield of cardiac immune cells. These isolated cardiac immune cells can then be used for characterization of functionality, phenotype, maturity, and co-culture experiments with other cardiac cells to gain a better understanding of their interactions.

This method for isolating functional immune cells from the heart provides an alternative to the conventional methods of collagenase digestion, which causes unwanted immune cell activation, resulting in a decreased responsiveness of these cells. Our method of isolation yields functional cardiac immune cells by avoiding problems associated with enzymatic digestion.

Cardiac immune cells are gaining interest for the roles they play in the pathological remodeling in many cardiac diseases.1-5  These immune cells, which ...

Intravital Imaging of the Mouse Thymus using 2-Photon Microscopy

Two-photon Microscopy (TPM) provides image acquisition in deep areas inside tissues and organs. In combination with the development of new stereotactic tools and surgical procedures, TPM becomes a powerful technique to identify "niches" inside organs and to document cellular "behaviors" in live animals. While intravital imaging provides information that best resembles the real cellular behavior inside the organ, it is both more laborious and technically demanding in terms of required equipment/procedures than alternative ex vivo imaging acquisition. Thus, we describe a surgical procedure and novel "stereotactic" organ holder that allows us to follow the movements of Foxp3+ cells within the thymus.
Foxp3 is the master regulator for the generation of regulatory T cells (Tregs). Moreover, these cells can be classified according to their origin: ie. thymus-differentiated Tregs are called "naturally-occurring Tregs" (nTregs), as opposed to peripherally-converted Tregs (pTregs). Although significant amount of research has been reported in the literature concerning the phenotype and physiology of these T cells, very little is known about their in vivo interactions with other cells. This deficiency may be due to the absence of techniques that would permit such observations. The protocol described in this paper provides a remedy for this situation.
Our protocol consists of using nude mice that lack an endogenous thymus since they have a punctual mutation in the DNA sequence that compromises the differentiation of some epithelial cells, including thymic epithelial cells. Nude mice were gamma-irradiated and reconstituted with bone marrows (BM) from Foxp3-KIgfp/gfp mice. After BM recovery (6 weeks), each animal received embryonic thymus transplantation inside the kidney capsule. After thymus acceptance (6 weeks), the animals were anesthetized; the kidney containing the transplanted thymus was exposed, fixed in our organ holder, and kept under physiological conditions for in vivo imaging by TPM. We have been using this approach to study the influence of drugs in the generation of regulatory T cells.

We have developed novel laboratory tools and protocols for intravital imaging acquisition of the thymus. Our technique should help in the identification of &#x201C;niches&#x201D; within the thymus where T cell development occurs.

Two-photon Microscopy (TPM) provides image acquisition in deep areas inside tissues and organs. In combination with the development of new stereotactic ...

Differentiating Functional Roles of Gene Expression from Immune and Non-immune Cells in Mouse Colitis by Bone Marrow Transplantation

To understand the role of a gene in the development of colitis, we compared the responses of wild-type mice and gene-of-interest deficient knockout mice to colitis. If the gene-of-interest is expressed in both bone marrow derived cells and non-bone marrow derived cells of the host; however, it is possible to differentiate the role of a gene of interest in bone marrow derived cells and non- bone marrow derived cells by bone marrow transplantation technique. To change the bone marrow derived cell genotype of mice, the original bone marrow of recipient mice were destroyed by irradiation and then replaced by new donor bone marrow of different genotype. When wild-type mice donor bone marrow was transplanted to knockout mice, we could generate knockout mice with wild-type gene expression in bone marrow derived cells. Alternatively, when knockout mice donor bone marrow was transplanted to wild-type recipient mice, wild-type mice without gene-of-interest expressing from bone marrow derived cells were produced. However, bone marrow transplantation may not be 100% complete. Therefore, we utilized cluster of differentiation (CD) molecules (CD45.1 and CD45.2) as markers of donor and recipient cells to track the proportion of donor bone marrow derived cells in recipient mice and success of bone marrow transplantation. Wild-type mice with CD45.1 genotype and knockout mice with CD45.2 genotype were used. After irradiation of recipient mice, the donor bone marrow cells of different genotypes were infused into the recipient mice. When the new bone marrow regenerated to take over its immunity, the mice were challenged by chemical agent (dextran sodium sulfate, DSS 5%) to induce colitis. Here we also showed the method to induce colitis in mice and evaluate the role of the gene of interest expressed from bone-marrow derived cells. If the gene-of-interest from the bone derived cells plays an important role in the development of the disease (such as colitis), the phenotype of the recipient mice with bone marrow transplantation can be significantly altered. At the end of colitis experiments, the bone marrow derived cells in blood and bone marrow were labeled with antibodies against CD45.1 and CD45.2 and their quantitative ratio of existence could be used to evaluate the success of bone marrow transplantation by flow cytometry. Successful bone marrow transplantation should show a vast majority of donor genotype (in term of CD molecule marker) over recipient genotype in both the bone marrow and blood of recipient mice.

Bone marrow transplantation provides a way to change the genotype of the bone marrow derived cells. If the gene of interest is expressed in both bone marrow derived cells and non-bone marrow derived cells, bone marrow transplantation can change the bone marrow derived cells to a different genotype without changing the non-bone marrow derived cell genotype.

To understand the role of a gene in the development of colitis, we compared the responses of wild-type mice and gene-of-interest deficient knockout mice ...

In vivo Imaging Method to Distinguish Acute and Chronic Inflammation

Inflammation is a fundamental aspect of many human diseases. In this video report, we demonstrate non-invasive bioluminescence imaging techniques that distinguish acute and chronic inflammation in mouse models. With tissue damage or pathogen invasion, neutrophils are the first line of defense, playing a major role in mediating the acute inflammatory response. As the inflammatory reaction progresses, circulating monocytes gradually migrate into the site of injury and differentiate into mature macrophages, which mediate chronic inflammation and promote tissue repair by removing tissue debris and producing anti-inflammatory cytokines. Intraperitoneal injection of luminol (5-amino-2,3-dihydro-1,4-phthalazinedione, sodium salt) enables detection of acute inflammation largely mediated by tissue-infiltrating neutrophils. Luminol specifically reacts with the superoxide generated within the phagosomes of neutrophils since bioluminescence results from a myeloperoxidase (MPO) mediated reaction. Lucigenin (bis-N-methylacridinium nitrate) also reacts with superoxide in order to generate bioluminescence. However, lucigenin bioluminescence is independent of MPO and it solely relies on phagocyte NADPH oxidase (Phox) in macrophages during chronic inflammation. Together, luminol and lucigenin allow non-invasive visualization and longitudinal assessment of different phagocyte populations across both acute and chronic inflammatory phases. Given the important role of inflammation in a variety of human diseases, we believe this non-invasive imaging method can help investigate the differential roles of neutrophils and macrophages in a variety of pathological conditions.

In vivo Imaging Method to Distinguish Acute and Chronic Inflammation

We describe a non-invasive imaging method for distinguishing inflammatory stages. Systemic delivery of luminol reveals areas of acute inflammation dependent upon MPO activity in neutrophils. In contrast, injection of lucigenin allows for visualization of chronic inflammation dependent upon Phox activity in macrophages.

Inflammation is a fundamental aspect of many human diseases. In this video report, we demonstrate non-invasive bioluminescence imaging techniques that ...

Generation of Lymph Node-fat Pad Chimeras for the Study of Lymph Node Stromal Cell Origin

The stroma is a key component of the lymph node structure and function. However, little is known about its origin, exact cellular composition and the mechanisms governing its formation. Lymph nodes are always encapsulated in adipose tissue and we recently demonstrated the importance of this relation for the formation of lymph node stroma. Adipocyte precursor cells migrate into the lymph node during its development and upon engagement of the Lymphotoxin-b receptor switch off adipogenesis and differentiate into lymphoid stromal cells (B&#233;n&#233;zech&#160;et al.14). Based on the lymphoid stroma potential of adipose tissue, we present a method using a lymph node/fat pad chimera that allows the lineage tracing of lymph node stromal cell precursors. We show how to isolate newborn lymph nodes and EYFP+ embryonic adipose tissue and make a LN/ EYFP+ fat pad chimera. After transfer under the kidney capsule of a host mouse, the lymph node incorporates local adipose tissue precursor cells and finishes its formation. Progeny analysis of EYFP+ fat pad cells in the resulting lymph nodes can be performed by flow-cytometric analysis of enzymatically digested lymph nodes or by immunofluorescence analysis of lymph nodes cryosections. By using fat pads from different knockout mouse models, this method will provide an efficient way of analyzing the origin of the different lymph node stromal cell populations.

Generation of lymph node/fat pad chimeras for the study of lymph node stromal cell origin is described. The method involves the isolation of lymph nodes from newborn mice and embryonic fat pads, the generation of chimeric lymph node-fat pads, and their transfer under the kidney capsule of a host mouse.

The stroma is a key component of the lymph node structure and function. However, little is known about its origin, exact cellular composition and the ...

Using Zebrafish Models of Human Influenza A Virus Infections to Screen Antiviral Drugs and Characterize Host Immune Cell Responses

Each year, seasonal influenza outbreaks profoundly affect societies worldwide. In spite of global efforts, influenza remains an intractable healthcare burden. The principle strategy to curtail infections is yearly vaccination. In individuals who have contracted influenza, antiviral drugs can mitigate symptoms. There is a clear and unmet need to develop alternative strategies to combat influenza. Several animal models have been created to model host-influenza interactions. Here, protocols for generating zebrafish models for systemic and localized human influenza A virus (IAV) infection are described. Using a systemic IAV infection model, small molecules with potential antiviral activity can be screened. As a proof-of-principle, a protocol that demonstrates the efficacy of the antiviral drug Zanamivir in IAV-infected zebrafish is described. It shows how disease phenotypes can be quantified to score the relative efficacy of potential antivirals in IAV-infected zebrafish. In recent years, there has been increased appreciation for the critical role neutrophils play in the human host response to influenza infection. The zebrafish has proven to be an indispensable model for the study of neutrophil biology, with direct impacts on human medicine. A protocol to generate a localized IAV infection in the Tg(mpx:mCherry) zebrafish line to study neutrophil biology in the context of a localized viral infection is described. Neutrophil recruitment to localized infection sites provides an additional quantifiable phenotype for assessing experimental manipulations that may have therapeutic applications. Both zebrafish protocols described faithfully recapitulate aspects of human IAV infection. The zebrafish model possesses numerous inherent advantages, including high fecundity, optical clarity, amenability to drug screening, and availability of transgenic lines, including those in which immune cells such as neutrophils are labeled with fluorescent proteins. The protocols detailed here exploit these advantages and have the potential to reveal critical insights into host-IAV interactions that may ultimately translate into the clinic.

Systemic and localized zebrafish infection models for human influenza A virus are demonstrated. Using a systemic infection model, zebrafish can be used to screen antiviral drugs. Using a localized infection model, zebrafish can be used to characterize host immune cell responses.

Each year, seasonal influenza outbreaks profoundly affect societies worldwide. In spite of global efforts, influenza remains an intractable healthcare ...

Quantifying Vibrio cholerae Colonization and Diarrhea in the Adult Zebrafish Model

Vibrio cholerae is best known as the infectious agent that causes the human disease cholera. Outside the human host, V. cholerae primarily exists in the aquatic environment, where it interacts with a variety of higher aquatic species. Vertebrate fish are known to be an environmental host and are a potential V. cholerae reservoir in nature. Both V. cholerae and the teleost fish species Danio rerio, commonly known as zebrafish, originate from the Indian subcontinent, suggesting a long-standing interaction in aquatic environments. Zebrafish are an ideal model organism for studying many aspects of biology, including infectious diseases. Zebrafish can be easily and rapidly colonized by V. cholerae after exposure in water. Intestinal colonization by V. cholerae leads to the production of diarrhea and the excretion of replicated V. cholerae. These excreted bacteria can then go on to colonize new fish hosts. Here, we demonstrate how to assess V. cholerae-intestinal colonization in zebrafish and how to quantify V. cholerae-induced zebrafish diarrhea. The colonization model should be useful to researchers who are studying whether genes of interest may be important for host colonization and/or for environmental survival. The quantification of zebrafish diarrhea should be useful to researchers studying any intestinal pathogen who are interested in exploring zebrafish as a model system.

Quantifying Vibrio cholerae Colonization and Diarrhea in the Adult Zebrafish Model

Zebrafish are a natural Vibrio cholerae host and can be used to recapitulate and study the entire infectious cycle from colonization to transmission. Here, we demonstrate how to assess V. cholerae colonization levels and quantify diarrhea in zebrafish.

Vibrio cholerae is best known as the infectious agent that causes the human disease cholera. Outside the human host, V. cholerae primarily exists in the ...

Modeling Tuberculosis in Mycobacterium marinum Infected Adult Zebrafish

Mycobacterium tuberculosis is currently the deadliest human pathogen causing 1.7 million deaths and 10.4 million infections every year. Exposure to this bacterium causes a wide disease spectrum in humans ranging from a sterilized infection to an actively progressing deadly disease. The most common form is the latent tuberculosis, which is asymptomatic, but has the potential to reactivate into a fulminant disease. Adult zebrafish and its natural pathogen Mycobacterium marinum have recently proven to be an applicable model to study the wide disease spectrum of tuberculosis. Importantly, spontaneous latency and reactivation as well as adaptive immune responses in the context of mycobacterial infection can be studied in this model. In this article, we describe methods for the experimental infection of adult zebrafish, the collection of internal organs for the extraction of nucleic acids for the measurement of mycobacterial loads and host immune responses by quantitative PCR. The in-house-developed, M. marinum-specific qPCR assay is more sensitive than the traditional plating methods as it also detects DNA from non-dividing, dormant or recently dead mycobacteria. As both DNA and RNA are extracted from the same individual, it is possible to study the relationships between the diseased state, and the host and pathogen gene-expression. The adult zebrafish model for tuberculosis thus presents itself as a highly applicable, non-mammalian in vivo system to study host-pathogen interactions.

Modeling Tuberculosis in Mycobacterium marinum Infected Adult Zebrafish

Here, we present a protocol to model human tuberculosis in an adult zebrafish using its natural pathogen Mycobacterium marinum. Extracted DNA and RNA from the internal organs of infected zebrafish can be used to reveal the total mycobacterial loads in the fish and the host&#39;s immune responses with qPCR.

Mycobacterium tuberculosis is currently the deadliest human pathogen causing 1.7 million deaths and 10.4 million infections every year. Exposure to this ...

Oral Intubation of Adult Zebrafish: A Model for Evaluating Intestinal Uptake of Bioactive Compounds

Most pathogens invade organisms through their mucosa. This is particularly true in fish as they are continuously exposed to a microbial-rich water environment. Developing effective methods for oral delivery of immunostimulants or vaccines, which activate the immune system against infectious diseases, is highly desirable. In devising prophylactic tools, good experimental models are needed to test their performance. Here, we show a method for oral intubation of adult zebrafish and a set of procedures to dissect and prepare the intestine for cytometry, confocal microscopy and quantitative polymerase chain reaction (qPCR) analysis. With this protocol, we can precisely administer volumes up to 50 &#181;L to fish weighing approximately 1 g simply and quickly, without harming the animals. This method allows us to explore the direct in vivo uptake of fluorescently labelled compounds by the intestinal mucosa and the immunomodulatory capacity of such biologics at the local site after intubation. By combining downstream methods such as flow cytometry, histology, qPCR and confocal microscopy of the intestinal tissue, we can understand how immunostimulants or vaccines are able to cross the intestinal mucosal barriers, pass through the lamina propria, and reach the muscle, exerting an effect on the intestinal mucosal immune system. The model could be used to test candidate oral prophylactics and delivery systems or the local effect of any orally administered bioactive compound.

The protocol describes intubating adult zebrafish with a biologic; then dissecting and preparing the intestine for cytometry, confocal microscopy and qPCR. This method allows administration of bioactive compounds to monitor intestinal uptake and the local immune stimulus evoked. It&#160;is relevant for testing the intestinal dynamics of oral prophylactics.