This work was supported by NICHD R00HD091386 to MLKW and by NIEHS T32ES027801 to AAE.

1&#160;Prepare the&#160;reagents and supplies
<ol>
	<li>Reagent preparation
	<ol>
		<li>Prepare 500 mL of 3x Danieau&#39;s solution (Solution 1, Table 1).</li>
		<li>Prepare 1 L of egg water (Solution 2, Table 1).</li>
		<li>Prepare a 1.2% solution of agarose in egg water. Melt the agarose entirely in the microwave, and then cool to 55 &#176;C in a water bath.</li>
		<li>Prepare 4 mL explant media (Solution 3, Table 1, modified slightly from19,21) per experimental condition. 
		NOTE: Remember to account for at least one well of explants from uninjected (or control injected) embryos when calculating the required volume.
		<ol>
			<li>Sanitize the workspace with 70% ethanol.</li>
			<li>Remove cell culture media from 4 &#176;C and spray/wipe with 70% ethanol.</li>
			<li>Make explant media and place in the 28.5 &#176;C incubator to warm while the embryos are injected. 
			NOTE: Always include age-matched, intact sibling embryos for staging purposes. Dechorionate these embryos and culture them on agarose-coated plates in 0.3x Danieau&#39;s solution (Solution 4, Table 1).</li>
		</ol>
		</li>
		<li>Remove pronase aliquots (1 mL at 20 mg/mL) from -20 &#176;C and allow to thaw on ice. Thaw one 1 mL aliquot for every three experimental conditions.</li>
	</ol>
	</li>
	<li>Prepare agarose plates
	<ol>
		<li>Make the injection plates.
		<ol>
			<li>Fill a 100 mm x 15 mm plastic Petri dish half-way&#160;with molten agarose in egg water.</li>
			<li>Gently place the injection mold on top of the molten agarose at a 45&#176; angle and lower it gradually into the agarose, ensuring that no bubbles are trapped underneath. Let it cool completely.</li>
			<li>Remove the mold. Use the plate immediately or save for later by adding 2 mL of egg water, wrapping the plate, and storing it at 4 &#176;C. Warm the plate for 15-30 min in the 28.5 &#176;C incubator before injection.</li>
		</ol>
		</li>
		<li>Make explant cutting plates.
		<ol>
			<li>Add 3 mL of molten 1.2% agarose in egg water to a 60 mm x 15 mm Petri dish, ensuring that the entire bottom of the well is coated. Let it cool completely.</li>
		</ol>
		</li>
		<li>Coat culture plates with agarose.
		<ol>
			<li>For each experimental condition, dispense 1 mL of molten 1.2% agarose in egg water into one well of a 6-well plate, ensuring that the entire bottom of the well is coated. Let it cool completely.</li>
		</ol>
		</li>
		<li>For making chimeric explants, create an explant cutting dish with small wells by adding twelve 1 mm glass beads to molten agarose in a 60 mm x 15 mm Petri dish. Remove the beads with forceps once the agarose cools&#160;completely.</li>
	</ol>
	</li>
</ol>
2 Inject embryos with RNA
<ol>
	<li>Wearing gloves, remove an aliquot of synthetic ndr2 mRNA from storage at -80 &#176;C and immediately place it on ice.</li>
	<li>Prepare the injection needle.
	<ol>
		<li>Fill a pulled glass capillary needle with RNA. Place the filled needle into a micro-manipulator and break the tip of the needle with forceps.</li>
		<li>Calibrate injection volume using a stage micrometer with a drop of mineral oil, adjusting injection time and pressure on the pneumatic injector to achieve a bolus of the desired size. A bolus with a diameter of 120 &#181;m has a volume of 1 nL. 
		NOTE: The desired volume of the bolus will depend on the concentration of the RNA and the desired dose per embryo. For example, if RNA is aliquoted at 10 ng/&#181;L, inject 1 nL to achieve a final amount of 10 pg.
		<ol>
			<li>Keep the RNA needle tip submerged in the oil until ready to inject.</li>
		</ol>
		</li>
	</ol>
	</li>
	<li>Load&#160;the embryos and inject.
	<ol>
		<li>Pull the dividers in breeding tanks, allow fish to spawn for 10-15 min, and collect the embryos using a tea strainer.</li>
		<li>Load the embryos into the injection plate using a Pasteur pipette and pipette pump, and then use a gloved finger to press the eggs into the troughs gently.</li>
		<li>Inject 10 pg ndr2 RNA into the yolk of single-cell embryos until the desired number of embryos is reached or until embryos begin to divide. 
		NOTE: Do not inject after the single-cell stage to ensure even distribution of the RNA throughout the embryo.</li>
		<li>Wash the embryos out of the injection plate into a labeled 100 mm x 15 mm Petri dish with a gentle stream of egg water from a squeeze bottle. 
		NOTE: Always keep a group of age-matched, uninjected siblings as controls.</li>
		<li>Place the embryos into the 28.5 &#176;C incubator until they reach the 128-cell stage. Remove unfertilized eggs and dead embryos from the dish.</li>
	</ol>
	</li>
</ol>
3 Dechorionate the embryos
<ol>
	<li>Once the embryos have reached the 128-cell stage, place them into labeled glass Petri dishes and decant as much egg water as possible from them.</li>
	<li>Label glass crystalizing dishes with lab tape (corresponding to small dish names) and fill 2/3 of the way with egg water. Place these dishes next to the dissecting microscope for quick accessibility.</li>
	<li>Add 1 mL of pronase stock (20 mg/mL, thawed on ice) to 15 mL of 3x Danieau&#39;s solution in a 50 mL conical tube. 
	NOTE: This amount is sufficient for up to three experimental conditions. Increase the volume of pronase and 3x Danieau&#39;s solution for additional explant conditions. 
	CAUTION: Pronase is an irritant; hence wear gloves when handling.</li>
	<li>Add at least 5 mL of pronase solution to each glass Petri dish containing embryos.</li>
	<li>Agitate the glass dishes in a circular motion, monitoring the progress of dechorionation consistently under a dissecting microscope.</li>
	<li>Once the chorions begin to wrinkle and 1-2 embryos are out of their chorions, carefully dunk the glass Petri dish containing pronase and the embryos into the corresponding glass crystallizing dish containing egg water.</li>
	<li>Wash the dechorionated embryos.
	<ol>
		<li>Wash the embryos three times with egg water by gently adding and then decanting egg water from the dish.</li>
		<li>The third and final wash is with 0.3x Danieau&#39;s solution. 
		&#8203;NOTE: If the embryos still have chorions after washing, gently pipette the embryos until the chorions are removed or let them sit in the wash (egg water or 0.3x Danieau&#39;s solution) for a minute or two and gently agitate with circular motions.</li>
	</ol>
	</li>
	<li>Cover dechorionated embryos with a Petri dish lid and return them to the incubator (28.5 &#176;C) until they reach the 256-cell stage.</li>
</ol>
4 Cut explants
<ol>
	<li>Fill the agarose-coated 60 mm x 15 mm Petri dish with 3x Danieau&#39;s solution.</li>
	<li>Once the embryos are at the 256-cell stage, transfer them into the agarose-coated plate containing 3x Danieau&#39;s solution, lining them up along the center of the dish.</li>
	<li>Cut the explants using forceps (Figure 1).
	<ol>
		<li>Use one pair of forceps, held closed, to stabilize the embryo and use the other to cut through the blastoderm at approximately half of its height (from margin to animal pole) (Figure 1A).</li>
		<li>To cut, gently squeeze the blastoderm cells with one pair of forceps. Then, take the stabilizing forceps and run them along the other forceps to slice approximately halfway across the blastoderm (Figure 1B).</li>
		<li>Rotate the embryo, placing the forceps into the existing cut, and then sever the remaining blastoderm orthogonal to the first cut (Figure 1C).</li>
	</ol>
	</li>
	<li>Keep explants in 3x Danieau&#39;s solution for at least 5 min to heal, then transfer them to the well of a 6-well plate coated with agarose and filled with 4 mL of explant media. 
	NOTE: Cut explants from uninjected (or control injected) siblings as negative controls. If explants are performed correctly, these explants will neither extend nor express markers of endoderm, mesoderm, or neuroectoderm.</li>
	<li>Place the explant culture plates into the 28.5 &#176;C incubator until the desired timepoint/stage (determined from intact siblings) is reached. 
	&#8203;NOTE: If treating explants with a compound, such as a small molecule inhibitor, the desired concentration can be added directly to the explant media within the wells at desired time points. Remember to include the volume of agarose when calculating concentrations. (Example: 1 mL agarose + 4 mL explant media = 5 mL total volume per well).</li>
</ol>
5 Prepare chimeric explants
<ol>
	<li>In place of a regular agarose coated plate, cut chimeric explants in a dish with agarose molded into twelve small, shallow wells using 1 mm glass beads (section 1.2.4). Fill this plate with 3x Danieau&#39;s solution. 
	&#8203;NOTE: Chimeric explants are generated from blastoderm cells of two embryos of different genotypes or conditions. Ensure that these conditions can be distinguished from one another by the expression of transgenic or injected fluorescent markers.
	<ol>
		<li>Prepare by adding twelve embryos of one genotype/condition to the left side of the plate and twelve embryos of the other genotype/condition to the right side of the plate.</li>
		<li>Move one embryo of each condition into the center of the plate, near one of the 12 wells.</li>
		<li>Using forceps, cut an explant from each embryo as described for single embryo explants (step 4.3).</li>
		<li>Quickly press the cut edges of the two explants together within the shallow well using forceps to allow the two halves to heal together into a single explant.</li>
		<li>Continue with the remaining eleven&#160;wells within the plate. Once explants are healed, transfer them to the well of a 6-well plate coated with agarose and filled with 4 mL of explant media. Repeat until the desired number of explants is achieved.</li>
	</ol>
	</li>
</ol>
6 Culture and/or image the fixed explants
<ol>
	<li>Culture explants in the 28.5 &#176;C incubator until intact sibling embryos reach the desired stage.</li>
	<li>Live explants can be mounted for continuous time-lapse imaging, imaged periodically throughout the culture period, or imaged live at the experimental endpoint.</li>
	<li>Fix the explants if desired. Once the explants reach the desired endpoint, note the stage of intact embryo siblings and place the explants into a glass scintillation vial with 1 mL of 4% paraformaldehyde in PBS. Fix overnight on a shaker at 4 &#176;C. 
	CAUTION: Paraformaldehyde is toxic. Wear gloves when handling this chemical and dispose of it via methods approved by each institution.
	<ol>
		<li>After fixation, rinse explants six times, 15 min each with PBS + 0.1% Tween-20, and dehydrate gradually into methanol. Store explants at -20 &#176;C for later analysis by the whole-mount in situ hybridization, immunofluorescent staining, etc.</li>
	</ol>
	</li>
</ol>

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<li>Veenvliet, J. V., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Mouse+embryonic+stem+cells+self-organize+into+trunk-like+structures+with+neural+tube+and+somites%5BTitle%5D)+AND+%22Science%22%5BJournal%5D)">Mouse embryonic stem cells self-organize into trunk-like structures with neural tube and somites.</a> Science. 370 (6522), (2020).</li>
<li>Beccari, L., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Multi-axial+self-organization+properties+of+mouse+embryonic+stem+cells+into+gastruloids%5BTitle%5D)+AND+%22Nature%22%5BJournal%5D)">Multi-axial self-organization properties of mouse embryonic stem cells into gastruloids.</a> Nature. 562 (7726), 272-276 (2018).</li>
<li>Moris, N., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((An+in+vitro+model+of+early+anteroposterior+organization+during+human+development%5BTitle%5D)+AND+%22Nature%22%5BJournal%5D)">An in vitro model of early anteroposterior organization during human development.</a> Nature. 582 (7812), 410-415 (2020).</li>
<li>vanden Brink, S. C., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Single-cell+and+spatial+transcriptomics+reveal+somitogenesis+in+gastruloids%5BTitle%5D)+AND+%22Nature%22%5BJournal%5D)">Single-cell and spatial transcriptomics reveal somitogenesis in gastruloids.</a> Nature. 582 (7812), 405-409 (2020).</li>
</ol>

The authors declare that they have no competing financial interests.

This article has described how to generate zebrafish blastoderm explants and discussed two practical applications of these explants in addressing the role of Nodal morphogen signaling in gastrulation. This method of cutting and culturing explants provides a blank slate of na&#239;ve cells that can be manipulated using RNA injections and treatment with small molecule compounds to investigate a molecular pathway of interest.
Critical steps 
There are four steps in this protocol that are particularly critical for its success. The first is injecting the embryos with the appropriate amount of Nodal. This protocol recommends 10 pg of ndr2 RNA, and although a range of doses promotes extension, too much or too little Nodal will prevent optimal explant extension20. The second step is dechorionating the embryos. If the embryos remain in pronase for too long, the yolks will burst, and the embryos will not be viable to cut. If they are not in the pronase long enough, the chorions will not be loosened by washing and will instead require time-consuming manual dechorionation. The third critical step is cutting the explants. Cutting in 3x Danieau&#39;s solution is recommended, as the lower salt content of 0.3x Danieau&#39;s solution or egg water does not promote healing and survival of explants.
Additionally, the explants must be cut at approximately half the height of the blastoderm to ensure the naivety of the cells. If they are cut too close to the yolk, they will contain signals from the margin (including endogenous Nodal) that promote tissue specification and morphogenesis. The fourth and final critical step is in the healing of chimeric explants. Two explants will not fuse to form chimeras unless their cut edges are gently pressed together immediately after they are cut.
Modifications and troubleshooting 
The critical steps described above provide opportunities for troubleshooting. Some common issues and proposed solutions are presented below.
If explants are not extending in the presence of Nodal signaling, there are some possible solutions. (A) Inject embryos at the single-cell stage to ensure that RNA is evenly dispersed throughout the entire embryo. (B) Avoid injecting too much nodal RNA by ensuring&#160;that the injected volume is correct using a micrometer to measure the injection bolus. (C) Avoid injecting too little nodal RNA by measuring its concentration to ensure it has not degraded. (D) Keep some age-matched intact siblings to infer the equivalent stage of the explants. Explants achieve maximum extension when intact siblings reach the 2-5 somite stage. If the explants are collected too early, then the optimal extension will not be reached.
If the yolks are bursting after dechorionation, and the embryos are not viable to cut, remove the embryos from pronase solution once the chorions begin to crinkle and 1-2 embryos shed their chorion. Then, rinse immediately in egg water.
If the explants appear bubbly around the edges, there are some solutions. (A) Cut explants only within a specific timeframe of development. Although explants cut at any stage from 128- to 1000-cell stages can survive and extend in culture, those cut at 256- to 512-cell stages tend to be the most robust. (B) Ensure that explants are cut in 3x Danieau&#39;s solution to ensure proper healing. (C) Cut explants cleanly but gently. Avoid stretching or pulling the cells apart during the cutting process.
If the uninjected control explants are extending, explants were likely to cut too close to the yolk. For explants to be na&#239;ve, ensure that the cuts are made halfway between the yolk and the top of the blastoderm.
If the chimeric explants fail to fuse, it is likely because the tendency of explants in 3x Danieau&#39;s solution once cut is to round up and heal over the cut edge. To ensure that the two blastoderms heal to each other rather than themselves, press them together immediately after cutting. Use forceps to apply gentle pressure to the newly joined blastoderms within the agarose well to encourage them to heal together.
Limitations 
While these explants are a valuable tool to study the role of a given morphogen (or another molecule of interest) in relative isolation, observations made in any ex vivo model must be interpreted with care. Explants exhibit C&#38;E morphogenesis that is very similar to that observed in vivo20, but they do not recapitulate all aspects of gastrulation, for example, epiboly movements. They also lack many other regulatory factors and signaling molecules that are present within an intact embryo. While this is a significant experimental advantage of explants, it can also lead to conclusions that do not hold in vivo. For example, since explants that do not receive exogenous Nodal ligands fail to express neuroectoderm markers, one might conclude from explants alone that Nodal signaling is required for neuroectoderm specification. However, neuroectoderm is formed within intact embryos lacking all Nodal signaling23,24, demonstrating the vital role of other signaling molecules in neural specification32. Explants can tell us what a morphogen is capable of&#160;in an isolated environment. Still, all such findings should be confirmed in/compared with intact embryos for results to be interpreted thoroughly. In other words, explants cannot take the place of a developing embryo. Instead, they are a supplementary tool to identify the role and relationship of a morphogen with the surroundings. With these limitations in mind, zebrafish blastoderm explants are a valuable tool for many research questions.
Significance with respect to existing methods 
With renewed interest in synthetic embryology, several ex vivo and in vitro approaches are regularly employed to model aspects of embryonic development. For example, 2- and 3-dimensional gastruloids composed of mouse or human embryonic / induced pluripotent stem cells can be coaxed, through the application of exogenous signaling molecules, to recapitulate some of the patterning&#160;and/or morphogenetic events of gastrulation, segmentation, and neurulation33,34,35,36,37. Although powerful, these methods require laborious and prolonged culture methods to both continuously maintain pluripotent stem cells and to grow gastruloids, which take many days to reach gastrulation stages. By contrast, zebrafish explants require no maintenance of stem cell cultures, as embryos are simply collected as needed. They are relatively simple to generate and reach gastrulation stages within hours, the same as zebrafish embryos. This highlights another advantage of zebrafish explants, their intact developmental clock. Because the developmental age of embryonic and induced pluripotent stem cells can be variable and highly debated, embryonic explants are perhaps better suited to investigate temporal regulation of development. Finally, while pescoid zebrafish explants (which contain the embryonic margin) similarly extend in culture12,13, they do so in response to endogenous signaling centers. Instead, the explants described here enable researchers to investigate molecules of interest with relatively little interference from such embryonic signals.
Potential future applications 
Here, explants were used to demonstrate that Nodal signaling is necessary and sufficient for C&#38;E morphogenesis. Still, it is anticipated that they can and will be used to discern the role of many different molecules in many other developmental processes, for example, regulation of gene expression, signaling gradients, and additional morphogenetic programs. Additionally, because these explants are viable until at least 24 hpf19, it can be expected that their utility will extend beyond gastrulation into processes such as segmentation and organogenesis, any process in which researchers desire a developmental blank slate.

A perennial goal of the developmental biology field is to unravel the complexity of developing embryos to understand the origin of animal form and function. Even early embryos contain a complex medley of signaling molecules, cell and tissue interactions, and mechanical forces, all subject to strict spatial and temporal regulation. For this reason, it is often challenging to pinpoint the precise role of a particular signal in a developmental process of interest. By removing embryonic tissues from their endogenous environment, embryo explantation creates a simplified platform in which to discern the developmental roles of individual tissues and molecules in relative isolation. Explantation techniques are perhaps best known in Xenopus laevis, where they have been used to study tissue induction, cell signaling, cell adhesion, and morphogenesis, among other processes1,2,3,4. So-called animal cap explants, in which the animal region of blastula stage Xenopus embryos is&#160;isolated before inductive interactions5,6,7, are a widespread and powerful explant technique. Unmanipulated animal caps are fated to become ectoderm7,8. Still, they are competent to respond to several inductive factors, allowing them to form tissues of all three germ layers and undergo tissue-appropriate morphogenetic movements9,10,11. However, limited genetic tools and sub-optimal suitability for live imaging prevent the use of Xenopus animal cap explants for many developmental biologists. By explanting blastoderm cells from zebrafish embryos, researchers can combine the utility of the animal cap assay with the optical clarity, abundance of genetic tools, and other experimental advantages of the zebrafish model system.
To date, researchers have made use of two flavors of zebrafish explants: so-called pescoids and the blastoderm explants. In the pescoid model, the entire blastoderm, including the marginal zone, is isolated from the yolk and allowed to develop ex vivo without the extraembryonic yolk syncytial layer (YSL)12,13. In this way, pescoids bear a notable resemblance to the Fundulus explants generated decades ago by Jane Oppenheimer and J.P. Trinkaus14,15. These explants recapitulate many aspects of embryonic patterning and morphogenesis12,13. However, because these isolates contain endogenous signaling centers (the embryonic margin), they are not simplified with regard to&#160;their molecular milieu. Alternatively, researchers can generate relatively na&#239;ve zebrafish blastoderm explants by excluding the marginal zone16,17,18,19,20,21. Unmanipulated zebrafish blastoderm explants express high levels of bone morphogenetic protein (BMP) morphogens19 and give rise to non-neural ectoderm and enveloping layer (EVL) when cultured ex vivo18. However, they recapitulate many aspects of axial patterning and morphogenesis in response to exogenous signaling gradients19,20,21, similar to Xenopus animal caps. For this reason, blastoderm explants are an advantageous model to study the role of a given morphogen (or morphogens) in germ layer specification, morphogenetic cell movements, and signaling gradients within a simplified signaling environment. Furthermore, blastoderms from embryos of different genotypes or conditions can be combined in a single chimeric explant19,21 to investigate cell/tissue autonomy and inductive interactions.
Zebrafish blastoderm explants can be used to investigate the role of embryonic signals (for example, Nodal) in morphogenesis and tissue specification during gastrulation. By injecting synthetic ndr2 RNA (encoding a Nodal ligand) at the single-cell stage, Nodal signaling is activated throughout the blastoderm of the embryo. Explants from these embryos generate Nodal signaling gradients, form all three germ layers, and undergo convergence and extension (C&#38;E) gastrulation movements as seen in intact embryos20. Additionally, chimeric explants are used to illustrate the ability of mesoderm tissues to induce neuroectoderm from uninjected (na&#239;ve) blastoderm. This protocol provides instructions for creating zebrafish blastoderm explants and demonstrates their utility in defining the role of Nodal signaling in tissue induction and morphogenesis.

<table><tbody><tr><td>1 mm glass beads</td><td>Millipore-Sigma</td><td>Z250473</td><td></td></tr><tr><td>4% Paraformaldehyde</td><td>VWR</td><td>J19943-K2</td><td></td></tr><tr><td>6-well plates</td><td>Fisher</td><td>FB012927</td><td></td></tr><tr><td>Agarose</td><td>Thermo-Fisher</td><td>16500500</td><td></td></tr><tr><td>Ca(NO&lt;sub&gt;3&lt;/sub&gt;)&lt;sub&gt;2 .&lt;/sub&gt;4H&lt;sub&gt;2&lt;/sub&gt;O</td><td>Thermo-Fisher</td><td>12364-36</td><td></td></tr><tr><td>DMEM/F12 media</td><td>Gibco</td><td>11330032</td><td></td></tr><tr><td>Dumont #5 watchmakers forceps</td><td>World Precision Instruments</td><td>500341</td><td></td></tr><tr><td>Embryo injection mold</td><td>Adaptive Science Tools</td><td>I-34</td><td></td></tr><tr><td>Glass crystalizing dishes</td><td>Fisher</td><td>08-741A</td><td></td></tr><tr><td>Glass Petri dishes</td><td>Fisher</td><td>08-748A</td><td></td></tr><tr><td>HEPES</td><td>VWR</td><td>JT4018-1</td><td></td></tr><tr><td>Instant Ocean sea salts</td><td>Instant Ocean</td><td>SS15-10</td><td></td></tr><tr><td>KCl</td><td>VWR</td><td>BDH9258-500G</td><td></td></tr><tr><td>Low temperature incubator</td><td>Fisher</td><td>15-015-2632</td><td></td></tr><tr><td>MgSO&lt;sub&gt;4.&lt;/sub&gt;7H&lt;sub&gt;2&lt;/sub&gt;O</td><td>VWR</td><td>97062-134</td><td></td></tr><tr><td>Microloader pipette tips</td><td>Eppendorf</td><td>930001007</td><td></td></tr><tr><td>Micromanipulator</td><td>World Precision Instruments</td><td>M3301R</td><td></td></tr><tr><td>Micrometer</td><td>SPI supplies</td><td>02265-AB</td><td></td></tr><tr><td>Mineral oil</td><td>VWR</td><td>MK635704</td><td></td></tr><tr><td>NaCl</td><td>VWR</td><td>BDH9286-500G</td><td></td></tr><tr><td>Newborn Calf Serum</td><td>Invitrogen</td><td>26010-066</td><td></td></tr><tr><td>Pasteur pipettes</td><td>Fisher</td><td>13-678-30</td><td></td></tr><tr><td>Penicillin-Streptomycin Solution</td><td>Thermo-Fisher</td><td>15140122</td><td></td></tr><tr><td>Pico-pump pneumatic injector</td><td>World Precision Instruments</td><td>SYS-PV820</td><td></td></tr><tr><td>Pipet pump</td><td>Fisher</td><td>13 683C</td><td></td></tr><tr><td>Plastic Petri dishes 100 mm</td><td>Fisher</td><td>FB0875712</td><td></td></tr><tr><td>Plastic Petri dishes 60 mm</td><td>Fisher</td><td>FB0875713A</td><td></td></tr><tr><td>Plastic wash bottles</td><td>Fisher</td><td>03-409-10E</td><td></td></tr><tr><td>Pronase</td><td>Millipore-Sigma</td><td>10165921001</td><td></td></tr><tr><td>Tween-20</td><td>VWR</td><td>200002-836</td><td></td></tr></tbody></table>

generation of na&#239;ve blastoderm explants from zebrafish embryos

Due to their optical clarity and rapid development, zebrafish embryos are an excellent system for examining cell behaviors and developmental processes. However, because of the complexity and redundancy of embryonic signals, it can be challenging to discern the complete role of any single signal during early embryogenesis. By explanting the animal region of the zebrafish blastoderm, relatively na&#239;ve clusters of embryonic cells are generated that can be easily cultured and manipulated ex vivo. By introducing a gene of interest by RNA injection before explantation, one can assess the effect of this molecule on gene expression, cell behaviors, and other developmental processes in relative isolation. Furthermore, cells from embryos of different genotypes or conditions can be combined in a single chimeric explant to examine cell/tissue interactions and tissue-specific gene functions. This article provides instructions for generating zebrafish blastoderm explants and demonstrates that a single signaling molecule - a Nodal ligand - is sufficient to induce germ layer formation and extension morphogenesis in otherwise na&#239;ve embryonic tissues. Due to their ability to recapitulate embryonic cell behaviors, morphogen gradients, and gene expression patterns in a simplified ex vivo system, these explants are anticipated to be of great utility to many zebrafish researchers.

Nodal ligands drive germ layer formation and C&#38;E of zebrafish blastoderm explants 
Control explants cut from uninjected wild-type (WT) embryos or those injected with 50 pg of mRNA encoding green fluorescent protein (GFP) remained rounded throughout the culture period (Figure 2A-C) and failed to express markers of mesoderm, endoderm, or neuroectoderm (Figure 3C)20. Together, these indicate an absence of the morphogenesis and germ layer formation that characterize vertebrate gastrulation. However, explants cut from embryos injected with 10 pg of ndr2 mRNA became highly elongated after 8-9 h in culture (Figure 2D). Live time-lapse imaging of these explants by differential interfering contrast (DIC) microscopy revealed that extension onsets at or around 8 h post-fertilization (hpf) (Figure 2F), the same time that C&#38;E morphogenesis begins in intact zebrafish embryos22. Explants cut from MZoep-/- embryos, which lack the essential tdgf1 Nodal co-receptor23, failed to extend in response to ndr2 injection (Figure 2E), demonstrating that Nodal activity is critical for this ex vivo morphogenesis. In addition, whole-mount in situ hybridization further showed that ndr2-expressing explants express markers of neuroectoderm (sox2) and several mesoderm sub-types (tbxta, noto, tbx16) (Figure 2G), as well as endoderm and the embryonic organizer20.
Nodal signaling is not required for neuroectoderm induction by mesoderm 
Nodal signaling activity is essential for induction of endoderm and most mesoderm but is dispensable for neuroectoderm specification within zebrafish gastrulae23,24. While uninjected zebrafish blastoderm explants did not differentiate into neuroectoderm (Figure 3C18), explants from embryos injected with 10 pg ndr2 exhibited robust expression of the neuroectoderm marker sox2 in distinct stripes along the long axis of the explant (Figure 2G), indicating that Nodal activity is required for neuroectoderm formation ex vivo. It has long been known that mesodermal tissues can induce neural tissue25,26,27,28,29, including in zebrafish blastoderm explants17. However, it is unclear whether neuroectoderm formation in this explant system requires Nodal signaling directly or whether exogenous Nodal ligands induce mesoderm that then induces&#160;neural tissues secondarily.
Chimeric explants containing&#160;prospective mesoderm and neuroectoderm portions from two different embryos were generated to test whether Nodal signaling is required tissue-autonomously for neuroectoderm specification ex vivo. The mesoderm portion of each explant was cut from an otherwise WT embryo expressing a mesoderm-specific transgenic GFP reporter, Tg[lhx1a:eGFP]30, injected with a high dose (100 pg) of ndr2 (Figure 3A). The putative neuroectoderm portion of each explant was cut from either a control WT embryo or Nodal signaling deficient MZoep-/- embryo injected only with mRNA encoding the fluorescent nuclear marker H2B-RFP (Figure 3A). Each chimeric explant was generated by combining one blastoderm from each of these two conditions, which were assayed for the expression of tissue-specific markers by whole-mount in situ hybridization at 12 hpf.
The majority of single-embryo explants from embryos injected with 100 pg ndr2 expressed little or no sox2, and expressed markers of mesoderm, including tbxta and the lhx1a:gfp reporter-throughout the explant (Figure 3B,G). Uninjected WT blastoderm (of the type that comprises the prospective neuroectoderm portion of chimeric explants) expressed neither mesoderm markers nor sox2 when cultured as a single explant, indicating a lack of neuroectoderm and mesoderm specification (Figure 3C,H). Single-embryo explants from MZoep-/- embryos similarly lacked expression of both neuroectoderm and mesoderm markers, even when injected with ndr2 (Figure 3D). However, when uninjected WT blastoderms were combined with mesoderm induced by high doses of Nodal ligands, these chimeric explants expressed both mesoderm markers and sox2 robustly (Figure 3E,I). These results demonstrate that, as previously observed17,26,27,29, mesoderm can induce neural fate in cells that would otherwise become non-neural ectoderm. To test whether Nodal signaling is required directly within the prospective neuroectoderm portion of these explants for their neural induction, chimeric explants were created from WT blastoderms injected with 100 pg ndr2 and blastoderms from MZoep-/- embryos (Figure 3J). Despite their inability to receive Nodal signals from the neighboring mesodermal portion, these explants expressed sox2 to a similar degree as WT control chimeras (Figure 3F). This result demonstrates that consistent with intact embryos in which neural tissues are specified in the absence of Nodal activity, Nodal signaling is not required tissue-autonomously for neuroectoderm induction ex vivo.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/62797/62797fig01.jpg" /> 
Figure 1: Procedure for zebrafish blastoderm explantation (step 4.3). (A) Hold the forceps in the non-dominant hand (orange) closed against the yolk to stabilize the embryo while pinching the blastoderm at approximately &#189; of its height using the forceps in the dominant hand (blue). (B) Run the orange forceps along the edge of the blue forceps gripping the embryo to slice through the blastoderm so that the first cut reaches approximately halfway across the blastoderm. (C) Rotate the embryo 90&#176;, then place the blue forceps inside (but orthogonal to) the original cut and pinch to sever the remaining blastoderm. (D) Allow explanted blastoderm cells to heal in 3x Danieau&#39;s solution for approximately 5 min before transferring into explant media. <a href="https://www.jove.com/files/ftp_upload/62797/62797fig01large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/62797/62797fig02.jpg" /> 
Figure 2&#160;(modified from20): Nodal ligands promote C&#38;E morphogenesis and germ layer formation in zebrafish blastoderm explants. (A) Diagram of injection and explantation of zebrafish embryos. (B-E) Representative bright-field images of live blastoderm explants of the indicated conditions/genotypes at the of equivalent the 2-4 somite stage. N = number of explants from two to four independent trials. (F) Time-lapse DIC series of a representative explant from a WT embryo injected with 10 pg ndr2 RNA. (G)Representative images of the whole-mount in situ hybridization for the transcripts indicated in explants from WT embryos injected with 10 pg ndr2 RNA. Scale bars are 200 &#181;m. <a href="https://www.jove.com/files/ftp_upload/62797/62797fig02large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/62797/62797fig03.jpg" /> 
Figure 3&#160;(Modified from31): Chimeric explants reveal that neuroectoderm specification does not require tissue-autonomous Nodal signaling ex vivo. (A) Diagram of the procedure to generate chimeric zebrafish explants. (B-F) Whole-mount in situ hybridization for the mesoderm marker tbxta (top) and neuroectoderm marker sox2 (bottom) in explants from WT embryos injected with 100 pg ndr2 RNA (B), uninjected WT controls (C), MZoep-/- injected with 10 pg ndr2 (D), and chimeric explants containing neuroectoderm portions from WT (E) or MZoep-/- (F) embryos at the equivalent of the 2-4 somite stage. Fractions indicate the number of explants with the phenotype shown over the total number of explants examined. (G-J) Representative images of live Tg[lhx1a:gfp] explants from a single embryo (G-H) or combined with H2B-expressing blastoderms (I-J, magenta) of the conditions indicated at the equivalent of the 2-4 somite stage. N = number of explants from three independent trials. Scale bars are 200 &#181;m. <a href="https://www.jove.com/files/ftp_upload/62797/62797fig03large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<table border="1" fo:keep-together.within-page="1" fo:keep-with-next.within-page="always">
	<tbody>
		<tr>
			<td></td>
			<td>Solution 1</td>
			<td>Solution 2</td>
			<td>Solution 3</td>
			<td>Solution 4</td>
		</tr>
		<tr>
			<td>Solution</td>
			<td>3x Danieau&#39;s</td>
			<td>Egg Water</td>
			<td>Explant Media</td>
			<td>0.3x Danieau&#39;s</td>
		</tr>
		<tr>
			<td>Ingredients</td>
			<td>174 mM NaCl</td>
			<td>60 &#181;g/mL sea salts</td>
			<td>DMEM/F12 + 2.5 mM L-Glutamine and 15 mM HEPES</td>
			<td>17.4 mM NaCl</td>
		</tr>
		<tr>
			<td></td>
			<td>2.1 mM KCl</td>
			<td>1 L distilled water</td>
			<td>3% total volume of Newborn Calf Serum or Fetal Bovine Serum</td>
			<td>0.21 mM KCl</td>
		</tr>
		<tr>
			<td></td>
			<td>1.2 mM MgSO4.7H2O</td>
			<td></td>
			<td>1:200 Penicillin (50 units/mL)-Streptomycin (50 &#181;g/mL)</td>
			<td>0.12 mM MgSO4&#8226;7H2O</td>
		</tr>
		<tr>
			<td></td>
			<td>1.8 mM Ca(NO3)2 &#8226;4H2O</td>
			<td></td>
			<td></td>
			<td>0.18 mM Ca(NO3)2 &#8226;4H2O</td>
		</tr>
		<tr>
			<td></td>
			<td>15 mM HEPES</td>
			<td></td>
			<td>Example:</td>
			<td>1.5 mM HEPES</td>
		</tr>
		<tr>
			<td></td>
			<td>Distilled water</td>
			<td></td>
			<td>4 mL/condition x 9 Conditions = 36 mL</td>
			<td>Distilled water</td>
		</tr>
		<tr>
			<td></td>
			<td></td>
			<td></td>
			<td>1.08 mL&#160;Newborn Calf Serum (NCS, aliquoted in -20 &#176;C (3%)</td>
			<td></td>
		</tr>
		<tr>
			<td></td>
			<td></td>
			<td></td>
			<td>0.18 mL&#160;200x Pen-Strep (PS, aliquoted in -20 &#176;C) (1:200)</td>
			<td></td>
		</tr>
		<tr>
			<td></td>
			<td></td>
			<td></td>
			<td>35 mL&#160;DMEM/F12</td>
			<td></td>
		</tr>
	</tbody>
</table>
Table 1.

Watch this Scientific Journal Video about Generation of NaÃ¯ve Blastoderm Explants from Zebrafish Embryos at JoVE.com

Generation of Na&#239;ve Blastoderm Explants from Zebrafish Embryos

Zebrafish blastoderm explants are generated by isolating embryonic cells from endogenous signaling centers within the early embryo, producing relatively na&#239;ve cell clusters easily manipulated and cultured ex vivo. This article provides instructions for making such explants and demonstrates their utility by interrogating roles for Nodal signaling during gastrulation.

Due to their optical clarity and rapid development, zebrafish embryos are an excellent system for examining cell behaviors and developmental processes. ...

generation-of-nave-blastoderm-explants-from-zebrafish-embryos

Nanyang Technological University

Research

JoVE Journal

Developmental Biology

3.3K Views.  Baylor College of Medicine. Zebrafish blastoderm explants are generated by isolating embryonic cells from endogenous signaling centers within the early embryo, producing relatively naïve cell clusters easily manipulated and cultured ex vivo. This article provides instructions for making such explants and demonstrates their utility by interrogating roles for Nodal signaling during gastrulation.

Video: Generation of Naïve Blastoderm Explants from Zebrafish Embryos

Microbead Implantation in the Zebrafish Embryo

The zebrafish has emerged as a valuable genetic model system for the study of developmental biology and disease. Zebrafish share a high degree of genomic conservation, as well as similarities in cellular, molecular, and physiological processes, with other vertebrates including humans. During early ontogeny, zebrafish embryos are optically transparent, allowing researchers to visualize the dynamics of organogenesis using a simple stereomicroscope. Microbead implantation is a method that enables tissue manipulation through the alteration of factors in local environments. This allows researchers to assay the effects of any number of signaling molecules of interest, such as secreted peptides, at specific spatial and temporal points within the developing embryo. Here, we detail a protocol for how to manipulate and implant beads during early zebrafish development.

The zebrafish is an excellent model system for genetic and developmental studies. Bead implantation is a valuable tissue manipulation technique that can be used to interrogate developmental mechanisms by introducing alterations in local cellular environments. This protocol describes how to perform microbead implantation in the zebrafish embryo.

The zebrafish has emerged as a valuable genetic model system for the study of developmental biology and disease. Zebrafish share a high degree of genomic ...

Generation of Parabiotic Zebrafish Embryos by Surgical Fusion of Developing Blastulae

Surgical parabiosis of two animals of different genetic backgrounds creates a unique scenario to study cell-intrinsic versus cell-extrinsic roles for candidate genes of interest, migratory behaviors of cells, and secreted signals in distinct genetic settings. Because parabiotic animals share a common circulation, any blood or blood-borne factor from one animal will be exchanged with its partner and vice versa. Thus, cells and molecular factors derived from one genetic background can be studied in the context of a second genetic background. Parabiosis of adult mice has been &#160;used extensively to research aging, cancer, diabetes, obesity, and brain development. More recently, parabiosis of zebrafish embryos has been used to study the developmental biology of hematopoiesis. In contrast to mice, the transparent nature of zebrafish embryos permits the direct visualization of cells in the parabiotic context, making it a uniquely powerful method for investigating fundamental cellular and molecular mechanisms. The utility of this technique, however, is limited by a steep learning curve for generating the parabiotic zebrafish embryos. This protocol provides a step-by-step method on how to surgically fuse the blastulae of two zebrafish embryos of different genetic backgrounds to investigate the role of candidate genes of interest. In addition, the parabiotic zebrafish embryos are tolerant to heat shock, making temporal control of gene expression possible. This method does not require a sophisticated set-up and has broad applications for studying cell migration, fate specification, and differentiation in vivo during embryonic development.

This protocol provides step-by-step instruction on how to generate parabiotic zebrafish embryos of different genetic backgrounds. When combined with the unparalleled imaging capabilities of the zebrafish embryo, this method provides a uniquely powerful means to investigate cell-autonomous versus non-cell-autonomous functions for candidate genes of interest.

Surgical parabiosis of two animals of different genetic backgrounds creates a unique scenario to study cell-intrinsic versus cell-extrinsic roles for ...

Generating Chimeric Zebrafish Embryos by Transplantation

One of the most powerful tools used to gain insight into complex developmental processes is the analysis of chimeric embryos. A chimera is defined as an organism that contains cells from more than one animal; mosaics are one type of chimera in which cells from more than one genotype are mixed, usually wild-type and mutant. In the zebrafish, chimeras can be readily made by transplantation of cells from a donor embryo into a host embryo at the appropriate embryonic stage. Labeled donor cells are generated by injection of a lineage marker, such as a fluorescent dye, into the one-cell stage embryo. Labeled donor cells are removed from donor embryos and introduced into unlabeled host embryos using an oil-controlled glass pipette mounted on either a compound or dissecting microscope. Donor cells can in some cases be targeted to a specific region or tissue of the developing blastula or gastrula stage host embryo by choosing a transplantation site in the host embryo based on well-established fate maps.

A step-by-step guide to generating targeted chimeric zebrafish embryos by transplantation at the blastula or gastrula stage.

One of the most powerful tools used to gain insight into complex developmental processes is the analysis of chimeric embryos. A chimera is defined as an ...

Biology

Transplantation of GFP-expressing Blastomeres for Live Imaging of Retinal and Brain Development in Chimeric Zebrafish Embryos

Cells change extensively in their locations and property during embryogenesis. These changes are regulated by the interactions between the cells and their environment. Chimeric embryos, which are composed of cells of different genetic background, are great tools to study the cell-cell interactions mediated by genes of interest. The embryonic transparency of zebrafish at early developmental stages permits direct visualization of the morphogenesis of tissues and organs at the cellular level. Here, we demonstrate a protocol to generate chimeric retinas and brains in zebrafish embryos and to perform live imaging of the donor cells. The protocol covers the preparation of transplantation needles, the transplantation of GFP-expressing donor blastomeres to GFP-negative hosts, and the examination of donor cell behavior under live confocal microscopy. With slight modifications, this protocol can also be used to study the embryonic development of other tissues and organs in zebrafish. The advantages of using GFP to label donor cells are also discussed. 

We demonstrate a protocol to generate chimeric zebrafish embryos for live imaging cellular behavior during embryogenesis.

Cells change extensively in their locations and property during embryogenesis. These changes are regulated by the interactions between the cells and their ...

A 3-D Tail Explant Culture to Study Vertebrate Segmentation in Zebrafish

Vertebrate embryos pattern their major body axis as repetitive somites, the precursors of vertebrae, muscle, and skin. Somites progressively segment from the presomitic mesoderm (PSM) as the tail end of the embryo elongates posteriorly. Somites form with regular periodicity and scale in size. Zebrafish is a popular model organism as it is genetically tractable and has transparent embryos that allow for live imaging. Nevertheless, during somitogenesis, fish embryos are wrapped around a large, rounding yolk. This geometry limits live imaging of PSM tissue in zebrafish embryos, particularly at higher resolutions that require a close objective working distance. Here, we present a flattened 3-D tissue culture method for live imaging of zebrafish tail explants. Tail explants mimic intact embryos by displaying a proportional slowdown of axis elongation and shortening of rostrocaudal somite lengths. We are further able to stall axis elongation speed through explant culture. This, for the first time, enables us to untangle the chemical input of signaling gradients from the mechanistic input of axial elongation. In future studies, this method can be combined with a microfluidic setup to allow time-controlled pharmaceutical perturbations or screening of vertebrate segmentation without any drug penetration concerns.

Here, we present the protocol for 3-D tissue culture of the zebrafish posterior body axis, enabling live study of vertebrate segmentation. This explant model provides control over axis elongation, alteration of morphogen sources, and subcellular resolution tissue-level live imaging.

Vertebrate embryos pattern their major body axis as repetitive somites, the precursors of vertebrae, muscle, and skin. Somites progressively segment from ...

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 ...

Preparation of Single-Somite Explants from Zebrafish Embryos

The body axis of vertebrate embryos is periodically subdivided into 3D multicellular units called somites. While genetic oscillations and molecular prepatterns determine the initial length-scale of somites, mechanical processes have been implicated in setting their final size and shape. To better understand the intrinsic material properties of somites, a method is developed to culture single-somite explant from zebrafish embryos. Single somites are isolated by first removing the skin of embryos, followed by yolk removal and sequential excision of neighboring tissues. Using transgenic embryos, the distribution of various sub-cellular structures can be observed by fluorescent time-lapse microscopy. Dynamics of explanted somites can be followed for several hours, thus providing an experimental framework for studying tissue-scale shape changes at single-cell resolution. This approach enables direct mechanical manipulation of somites, allowing for dissection of the material properties of the tissue. Finally, the technique outlined here can be readily extended for explanting other tissues such as the notochord, neural plate, and lateral plate mesoderm.

We present a protocol for isolating single somites from zebrafish embryos, the dynamics of which can be followed in culture for several hours by fluorescence time-lapse microscopy, thus providing a methodology to quantify tissue-scale shape changes at single-cell resolution.

The body axis of vertebrate embryos is periodically subdivided into 3D multicellular units called somites. While genetic oscillations and molecular ...

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 ...

Blastomere Explants to Test for Cell Fate Commitment During Embryonic Development

Fate maps, constructed from lineage tracing all of the cells of an embryo, reveal which tissues descend from each cell of the embryo. Although fate maps are very useful for identifying the precursors of an organ and for elucidating the developmental path by which the descendant cells populate that organ in the normal embryo, they do not illustrate the full developmental potential of a precursor cell or identify the mechanisms by which its fate is determined. To test for cell fate commitment, one compares a cell's normal repertoire of descendants in the intact embryo (the fate map) with those expressed after an experimental manipulation. Is the cell's fate fixed (committed) regardless of the surrounding cellular environment, or is it influenced by external factors provided by its neighbors? Using the comprehensive fate maps of the Xenopus embryo, we describe how to identify, isolate and culture single cleavage stage precursors, called blastomeres. This approach allows one to assess whether these early cells are committed to the fate they acquire in their normal environment in the intact embryo, require interactions with their neighboring cells, or can be influenced to express alternate fates if exposed to other types of signals.

The fate of an individual embryonic cell can be influenced by inherited molecules and/or by signals from neighboring cells. Utilizing fate maps of the cleavage stage Xenopus embryo, single blastomeres can be identified for culture in isolation to assess the contributions of inherited molecules versus cell-cell interactions.

Fate maps, constructed from lineage tracing all of the cells of an embryo, reveal  which tissues descend from each cell of the embryo.  Although fate maps ...

Production of Haploid Zebrafish Embryos by In Vitro Fertilization

The zebrafish has become a mainstream vertebrate model that is relevant for many disciplines of scientific study. Zebrafish are especially well suited for forward genetic analysis of developmental processes due to their external fertilization, embryonic size, rapid ontogeny, and optical clarity &#8211; a constellation of traits that enable the direct observation of events ranging from gastrulation to organogenesis with a basic stereomicroscope. Further, zebrafish embryos can survive for several days in the haploid state. The production of haploid embryos in vitro is a powerful tool for mutational analysis, as it enables the identification of recessive mutant alleles present in first generation (F1) female carriers following mutagenesis in the parental (P) generation. This approach eliminates the necessity to raise multiple generations (F2, F3, etc.) which involves breeding of mutant families, thus saving the researcher time along with reducing the needs for zebrafish colony space, labor, and the husbandry costs. Although zebrafish have been used to conduct forward screens for the past several decades, there has been a steady expansion of transgenic and genome editing tools. These tools now offer a plethora of ways to create nuanced assays for next generation screens that can be used to further dissect the gene regulatory networks that drive vertebrate ontogeny. Here, we describe how to prepare haploid zebrafish embryos. This protocol can be implemented for novel future haploid screens, such as in enhancer and suppressor screens, to address the mechanisms of development for a broad number of processes and tissues that form during early embryonic stages.

Production of Haploid Zebrafish Embryos by In Vitro Fertilization

The zebrafish is a powerful model system for developmental biology and human disease research due to their genetic similarity with higher vertebrates. This protocol describes a methodology to create haploid zebrafish embryos that can be utilized for forward screen strategies to identify recessive mutations in genes essential for early embryogenesis.

The zebrafish has become a mainstream vertebrate model that is relevant for many disciplines of scientific study. Zebrafish are especially well suited for ...

Generation of Naïve Blastoderm Explants from Zebrafish Embryos

Summary

Explore More Videos

Microbead Implantation in the Zebrafish Embryo

Generation of Parabiotic Zebrafish Embryos by Surgical Fusion of Developing Blastulae

Generating Chimeric Zebrafish Embryos by Transplantation

Transplantation of GFP-expressing Blastomeres for Live Imaging of Retinal and Brain Development in Chimeric Zebrafish Embryos

A 3-D Tail Explant Culture to Study Vertebrate Segmentation in Zebrafish

A Simple and Effective Transplantation Device for Zebrafish Embryos

Preparation of Single-Somite Explants from Zebrafish Embryos

High-resolution Cell Transplantation in Embryonic and Larval Zebrafish

Blastomere Explants to Test for Cell Fate Commitment During Embryonic Development

Production of Haploid Zebrafish Embryos by In Vitro Fertilization