<em>In Situ</em> Hybridization in Zebrafish Larvae and Juveniles during Mesonephros Development

Sagar N. Kasar; Sarah A. Grandinette; Scott D. Semelsberger; Cuong  Q. Diep

doi:10.3791/62930

JoVE Journal > Developmental Biology

Developmental Biology

In Situ Hybridization in Zebrafish Larvae and Juveniles during Mesonephros Development

Published: August 13, 2021

doi:

10.3791/62930

Sagar N. Kasar¹, Sarah A. Grandinette¹, Scott D. Semelsberger¹, Cuong Q. Diep¹

¹Department of Biology,Indiana University of Pennsylvania

Summary

The zebrafish is an important model for understanding kidney development. Here, an in situ hybridization protocol is optimized to detect gene expression in zebrafish larvae and juveniles during mesonephros development.

Abstract

The zebrafish forms two kidney structures in its lifetime. The pronephros (embryonic kidney) forms during embryonic development and begins to function at 2 days post fertilization. Consisting of only two nephrons, the pronephros serves as the sole kidney during larval life until more renal function is required due to the increasing body mass. To cope with this higher demand, the mesonephros (adult kidney) begins to form during metamorphosis. The new primary nephrons fuse to the pronephros and form connected lumens. Then, secondary nephrons fuse to primary ones (and so on) to create a branching network in the mesonephros. The vast majority of research is focused on the pronephros due to the ease of using embryos. Thus, there is a need to develop techniques to study older and larger larvae and juvenile fish to better understand mesonephros development. Here, an in situ hybridization protocol for gene expression analysis is optimized for probe penetration, washing of probes and antibodies, and bleaching of pigments to better visualize the mesonephros. The Tg(lhx1a-EGFP) transgenic line is used to label progenitor cells and the distal tubules of nascent nephrons. This protocol fills a gap in mesonephros research. It is a crucial model for understanding how new kidney tissues form and integrate with existing nephrons and provide insights into regenerative therapies.

Introduction

The zebrafish embryo is an important model for studying tissue development due to its small size, transparency, available tools, and survival without feeding for up to five days¹^,². It has greatly contributed to the understanding of kidney development and the conservation between zebrafish and mammals³^,⁴^,⁵. The kidney plays an essential role in maintaining fluid homeostasis, filtering the blood, and excreting waste⁶. The nephron, the functional unit of the kidney, comprises a blood filter connected to a long tubule. In zebrafish, two kidney structures form throughout its life. The pronephros (the temporary embryonic kidney) forms first during early development. It consists of two nephrons running along the anterior-posterior axis and becomes functional at around 2 days post fertilization (dpf). The utility of the pronephros lies in its simplicity, having just two nephrons that are mostly linear and easy to visualize (although the proximal convoluted tubule begins to coil at three dpf)³. This has facilitated not only studies of its early development from the intermediate mesoderm, but also the segmentation pattern and tubule repair⁷^,⁸.

The usefulness of zebrafish becomes limited after five dpf, when the yolk is diminished and the larvae rely on feeding in the aquatic system⁹. At around 2 weeks old, the larvae undergo metamorphosis into juveniles, where new tissues form and old tissues are lost and/or reorganized⁹. This is also when the mesonephros (the permanent adult kidney) forms¹⁰^,¹¹^,¹². The first adult nephron forms near the sixth somite, and fuses with the distal early tubule of the pronephros. Additional nephrons are added posterior to this position initially, but also toward the anterior later on. The primary nephrons in this first wave fuse to the tubules of the pronephros and share a common lumen to deposit their waste. Secondary nephrons form in the next wave and fuse to primary nephrons. This reiterative process creates a mesonephros that is branched, somewhat akin to the mammalian kidney. Presumably, the pronephros eventually loses its tubule identity and becomes two major collecting ducts where all nephrons drain their waste¹³.

Prior to the formation of the first adult nephron, single progenitor cells begin to appear in ~4 mm (total length) larvae (~10 dpf). These cells, which are marked in the Tg(lhx1a-EGFP) transgenic line, adhere to the pronephros and seem to migrate to future sites of nephrogenesis. The single cells coalesce into clusters, which differentiate into new nephrons¹². It is unclear where these cells reside or what genes they express before the onset of mesonephrogenesis.

Understanding mesonephros development provides insights into the mammalian kidney in ways that the pronephros cannot. These include the formation of nephrogenic aggregates from single progenitor cells, functional integration of new nephrons with existing ones, and branching morphogenesis. However, there are limitations to studying postembryonic development. The larvae are less transparent due to their larger size and having pigmentation. The developmental timeline is not synchronous among individual animals and is highly dependent on environmental factors, such as feeding and crowding⁹^,¹⁴. Although knockdown reagents exist, they are less effective in larvae compared to embryos¹⁵. In this protocol, an in situ hybridization method to determine gene expression during zebrafish mesonephros development is described. Several steps are optimized to increase visualization of the mesonephros and penetration and washing of the probe and antibody. The Tg(lhx1a-EGFP) transgenic line is used along with a probe for EGFP to label single progenitor cells, nephrogenic aggregates, and the distal tubules of nascent nephrons. This method will provide a deeper understanding of mesonephros development and insight into regenerative therapies.

Protocol

The use of zebrafish larvae and juveniles is approved by the IUP IACUC (protocol #02-1920, #08-1920). Details of the solution content are listed in the Table of Materials.

1. Raising larvae

NOTE: It will take up to 21 days or more to raise larvae and juveniles to the stage of interest.

Set up adult zebrafish to mate by adding 1 male and 1 female fish in a mating tank in the late afternoon after their last meal.
NOTE: Not all fish pairs will mate. Start by setting up 20 pairs to determine the mating rate and adjust accordingly in future experiments.
The next day after the fish have finished mating (around 1 pm), collect the embryos with E3 medium in Petri plates.
1. Ensure that there are no more than 30 embryos per plate.
2. Remove debris (such as feces) from the Petri plates and add 20 mL of E3 medium.
3. Incubate at 28.5 °C for 1 day.
Put the adult zebrafish back in the aquatic system.
At 1 dpf, replace the E3 medium with fresh E3.
1. Incubate at 28.5 °C for 4 more days until 5 dpf.
Put a 400 µm screen in a 2.8 L tank and fill it with 2 cm of system water.
1. Add the 5 dpf larvae from 1 plate (up to 30 total larvae).
2. Put the tank in the aquatic system, but do not start the water flow.
Feed the larvae 4 mL of powder food twice a day until 14 dpf.
At 6 dpf, start the water flow at 1 drip per second.
NOTE: Check the waterflow daily and adjust accordingly.
At 8 dpf, increase the water flow to a slow, steady stream.
At 14 dpf, feed live brine shrimp in addition to the powder food.

2. Day 1 – 2: Fixing larvae

Remove a tank of larvae at the desired timepoint.
Fill a Petri plate with 20 mL of system water.
Use a fine mesh net to gently scoop the larvae and bring them to the water surface.
1. Cut off the tip of a transfer pipette to give a wider opening and transfer the larvae to the Petri plate. The larger pipette mouth allows for the transfer of several small larvae or a few larger ones at once.
Add 2 mL of tricaine (2%, pH 7 stock) to immobilize the larvae.
1. After the larvae stop moving, remove most of the water and add 10 mL of tricaine. Wait for 15 min for the larvae to be euthanized.
2. Optional: For juveniles longer than 8 mm, cut off the heads and tails with a razor blade (after euthanasia) under a dissecting microscope to improve penetration of the fixing solution. Make sure to record the total length of each animal before cutting off the head and tail and isolate each one in its own Petri plate. Refer to step 3 for how to measure the animals.
Replace the tricaine with 20 mL of fixing solution (4% paraformaldehyde, 1% DMSO). Put the lid back on the Petri plate and rock slowly in a fume hood.
NOTE: It is important to use a rocking platform. A shaking platform with a circular motion will cause the animal axis to be curved. Use only fresh (not premade frozen) fixing solution.
CAUTION: The fixing solution contains paraformaldehyde, which is a probable carcinogen. Use fume hood (or mask) and gloves to measure the powder.
After 30 min, replace the fixing solution with a fresh fixing solution.
1. Collect the used fixing solution in a separate waste container for proper disposal.
2. Transfer the larvae into a 50 mL tube containing 25 mL of fresh fixing solution.
3. Make sure the cap is tight and rock slowly at 4 °C for 2 days. It is possible to incubate longer for convenience.

3. Day 3: Measuring larvae

In a fume hood, replace the fixing solution with 20 mL of PBST.
Transfer the larvae into a Petri plate.
Put a flat ruler on a dissecting microscope and put the Petri plate on top of the ruler.
Use an eyelash manipulator to move each larva onto the ruler to measure its total length (from the snout to the tip of the caudal fin) (Figure 1).
Combine several larvae of similar lengths (e.g., 5.0 mm and 5.1 mm) into one 5.5 mL glass vial, up to 10 larvae per vial.

4. Day 3 – 4: Dehydration

Replace the PBST with 4 mL of 100% methanol. Rock the vial for 5 min at room temperature.
Replace the methanol with fresh methanol and rock for 5 min. Repeat one more time.
Store the vial at -20 °C for 2 days. It is possible to incubate longer for convenience.

5. Day 5: Rehydration

Warm the vial to room temperature.
Replace the methanol with 4 mL of 75% methanol/25% PBST. Rock for 5 min at room temperature.
Replace the solution in step 5.2 with 4 mL of 50% methanol/50% PBST and rock for 5 min.
Replace the solution in step 5.3 with 4 mL of 25% methanol/75% PBST and rock for 5 min.
Replace the solution in step 5.4 with 4 mL PBST and rock for 10 min.
Replace the PBST with 4 mL of fresh PBST and rock for 10 min. Repeat one more time.

6. Day 5: Proteinase K digest

Replace the PBST with 2 mL of the proteinase K solution (20 µg/mL, 1% DMSO final concentration in PBST) and rock at room temperature for 30 min.
NOTE: Larvae longer than 6 mm will need a longer incubation time and/or a higher proteinase K concentration. The exact time and concentration will need to be determined empirically. Start with a 10 min increase in incubation time for every 0.5 mm longer than 6 mm.
Replace the proteinase K solution with 4 mL of PBST and rock for 10 min.
Replace the PBST with 4 mL of fresh PBST and rock for 10 min. Repeat one more time.
Replace the PBST with 4 mL of fresh fixing solution and rock for 1 h. It is possible to incubate longer at 4 °C for convenience.

7. Day 5: Bleaching

Replace the fixing solution with 4 mL of PBST and rock at room temperature for 10 min.
Replace the PBST with 4 mL of fresh PBST and rock for 10 min. Repeat one more time.
Transfer the larvae to a 6-well plate (up to 10 larvae per well).
Replace the PBST with 3 mL of fresh bleaching solution.
Rock at room temperature and monitor the pigmentation under a dissecting microscope every 5 min. Look for the disappearance of pigmentation along the mesonephros (dorsal to the swim bladder and gut).
NOTE: For larvae up to 6 mm long, it will take up to 20 min to bleach the pigmentation surrounding the mesonephros. Do not bleach longer than necessary to preserve the integrity of the larvae.
Transfer the larvae back into a glass vial.
Replace the bleaching solution with 4 mL of PBST. Rock for 10 min.
Replace the PBST with 4 mL of fresh PBST and rock for 10 min. Repeat one more time.
Replace the PBST with 4 mL of fresh fixing solution and rock for 1 h. It is possible to incubate longer at 4 °C for convenience.

8. Day 5: Prehybridization

NOTE: For steps done at 70 °C, it is important to work quickly to minimize the vial cooling down.

Replace the fixing solution with 4 mL of PBST and rock at room temperature for 10 min.
Replace the PBST with 4 mL of fresh PBST and rock for 10 min. Repeat one more time.
Replace the PBST with 4 mL of the Hyb- solution, and rock at room temperature for 10 min.
CAUTION: The Hyb-, Hyb+, and probe solutions contain formamide, which can irritate the skin. Use gloves to handle these solutions.
Replace the Hyb- with 4 mL of fresh Hyb- and rock for 10 min. Repeat one more time.
1. Collect the used Hyb-, Hyb+, and probe solutions in a separate waste container for proper disposal.
Replace the Hyb- with 4 mL of the Hyb+ solution.
Incubate the vial at 70 °C overnight.
Dilute the EGFP-fluorescein probe 1:100 in 500 µL of Hyb+ and incubate it O/N at 70 °C.
NOTE: Follow the manufacturer's instructions for probe synthesis.

9. Day 6: Probe hybridization

Replace the Hyb+ solution in the vial with the preheated probe and incubate at 70 °C overnight.
NOTE: Larvae longer than 6 mm need 2 days of incubation.
Preheat the wash buffer, 2x SSCT, and 0.2x SSCT solutions at 70 °C for overnight.

10. Day 7: Probe washing

Replace the probe with 4 mL of the preheated wash buffer and incubate at 70 °C for 30 min.
1. Collect the used probe in a separate waste container for proper disposal.
Replace the wash buffer with 4 mL of fresh wash buffer and incubate at 70 °C for 30 min.
Replace the wash buffer with 4 mL of the preheated 2x SSCT solution and incubate it at 70 °C for 15 min.
Add 50 mL of preheated 0.2x SSCT into a 50 mL tube.
1. Insert a cell strainer (100 µm) into the top of the tube. Ensure that the cell strainer is pushed all the way down until it stops.
2. Transfer the larvae from the glass vial into the cell strainer. Ensure that the larvae are submerged in the buffer and incubate at 70 °C for 2 h.
Prepare a new tube containing 50 mL of preheated 0.2x SSCT.
1. Transfer the cell strainer from step 10.4.2 into the new tube of 0.2x SSCT and incubate at 70 °C for 2 h.
2. Repeat step 10.5 one more time.

11. Day 7: Blocking

Transfer the larvae to a new glass vial and cool to room temperature.
Replace the 0.2x SSCT with 4 mL of 67% 0.2x SSCT/33% MABT and rock at room temperature for 10 min.
Replace the solution in step 11.2 with 4 mL of 33% 0.2x SSCT/67% MABT and rock for 10 min.
Replace the solution in step 11.3 with 4 mL of MABT and rock for 10 min.
Replace the MABT with 4 mL of fresh MABT and rock for 10 min. Repeat one more time.
Replace the MABT with 4 mL of the blocking solution and incubate at 4 °C overnight. It is possible to incubate longer for convenience.

12. Day 8 – 9: Antibody incubation

Dilute the anti-fluorescein antibody 1:5,000 in 500 µL blocking solution.
Replace the blocking solution with the antibody solution and incubate at 4 °C for 2 days. It is possible to incubate longer for convenience.
1. Swirl the vial twice a day to agitate the larvae.
  NOTE: Larvae longer than 6 mm need 1-2 more days of incubation.

13. Day 10 – 11: Antibody washing

Replace the antibody solution with 4 mL of PBST and rock at room temperature for 10 min.
Replace the PBST with 4 mL of fresh PBST and rock for 10 min. Repeat one more time.
Transfer the larvae into a 50 mL tube.
Add 40 mL of PBST2. Lay the tube on its side and rock at 4 °C overnight.
Replace the PBST2 with 40 mL of fresh PBST2 and rock at 4 °C overnight. It is possible to incubate longer for convenience.
NOTE: Larvae longer than 6 mm need 1-2 more days of washing.

14. Day 12: Staining

Transfer the larvae to a 6-well plate.
Replace the PBST2 with 3 mL of staining buffer and rock at room temperature for 5 min.
Replace the staining buffer with 3 mL of fresh staining buffer and rock for 5 min. Repeat one more time.
Replace the staining buffer with 3 mL of the staining solution. Cover with aluminum foil and monitor the staining over the next few hours.
1. For probes with a weak signal, incubate at 4 °C overnight and replace the staining solution with fresh staining solution once in between.
When the desired staining intensity is reached, replace the staining solution with 3 mL of the stopping solution and rock for 30 min.
Replace the stopping solution with 3 mL of fresh stopping solution and rock for 30 min. Repeat one more time.
Transfer the larvae to a new glass vial and replace the stopping solution with 4 mL of fresh fixing solution and incubate for 1 h at room temperature. It is possible to incubate longer at 4 °C for convenience.
Store the larvae in the fixing solution in the dark at 4 °C for up to a year.

15. Day 12: Imaging

Replace the fixing solution with 4 mL of PBST and rock at room temperature for 10 min.
Transfer the larvae to a 6-well plate.
Replace the PBST with 4 mL of fresh PBST and rock for 10 min. Repeat one more time.
Replace the PBST with 3 mL of 50% glycerol (in PBST) and rock for 10 min.
Replace the solution in step 15.4 with 3 mL of 100% glycerol with no rocking for 10 min.
Use a dissecting microscope to image the larvae directly in the 6-well plate or transfer the larvae into a depression slide to image under a compound microscope. Use an eyelash manipulator to orient the larvae.

Representative Results

Using the Tg(lhx1a-EGFP) transgenic line, it was demonstrated that this in situ hybridization protocol is effective in labeling kidney progenitor cells and various nephron structures during mesonephros development. As expected, the central nervous system is also labeled in this transgenic line (not shown). The initial mesonephric nephron forms at approximately 5.2 mm, dorsal to the pronephros (Figure 2A), and the distal tubule of this nephron is labeled by EGFP¹⁰^,¹². Progenitor clusters are present at this stage and later on (Figure 2A–B, arrowheads), and single progenitor cells are also labeled (Figure 2C). This method provides an additional tool in studying kidney development and helps shed light on understanding the human kidney.

Figure 1: Measuring larvae. Fixed larvae in a Petri plate are placed on top of a flat ruler. Under a dissecting microscope, the larvae are measured and separated by groups of similar sizes. Please click here to view a larger version of this figure.

Figure 2: Mesonephros development. At around 5.2 mm in the Tg(lhx1a-EGFP) transgenic line, the first mesonephric nephron is formed dorsal to pronephros and swim bladder (SB) (A). Clusters of progenitor cells are present during mesonephros development (A–B, arrowheads) in addition to single progenitor cells (C, bracket). In larger juveniles, background staining can occur in the somites (C, arrows). Please click here to view a larger version of this figure.

Discussion

The in situ hybridization method described here is aimed toward studying mesonephros development. However, it can be applied to study the development of other tissues and organs during metamorphosis, such as the gut, nervous system, scales, and pigmentation¹⁴. Probes can be generated for endogenous genes or fluorescent markers in transgenic lines.

It is critical for the larvae to remain intact in order to observe the organs and tissues in their native context. To retain tissue integrity, it is important to minimize the time of proteinase K treatment. It is important to determine the best treatment time for each new batch of enzyme. Alternatively, acetone can be used instead of proteinase K for improved tissue integrity¹⁶. Excessive bleaching also reduces tissue integrity. Minimal bleaching and allowing the eyes to retain some pigmentation help in visualizing the larvae during washes. It is common for the eyes to fall off during the hybridization step, which is an indicator of tissue fragility. The use of DMSO with the fixing and proteinase K solution is crucial for tissue penetration¹⁷.

A limitation of this method is the poor penetration of reagents in larger animals. To improve penetration, the head and tail can be removed with a razor blade before fixation¹⁷. The gut can be removed with fine tweezers and tungsten needles after fixation to allow direct access of the reagents to the mesonephros. Long probes (greater than 1 KB) can have poor penetration of the tissue, but they can be hydrolyzed into short fragments (around 0.3 KB) to improve penetration¹⁸. For probes with weak signals, control probes with the sense sequence can be used to differentiate between the background and the probe signal. Larger animals will have a higher background staining of the somites (Figure 2C, arrows). However, this can be minimized with longer washes of the probe and antibodies.

The protocol here can also be applied to dissected and isolated tissues and organs, such as the adult zebrafish kidney¹²^,¹⁹. Although there are published descriptions of similar protocols⁹^,¹⁶, none of them describe the entire process from rearing larvae to in situ hybridization with this level of detail. Therefore, this method provides an additional tool in deciphering the development of the vertebrate kidney.

Disclosures

The authors have nothing to disclose.

Acknowledgements

Funding was provided by the Pennsylvania Academy of Science, and the Commonwealth of Pennsylvania Biologists, and the Indiana University of Pennsylvania (School of Graduate Studies and Research, Department of Biology, and the Cynthia Sushak Undergraduate Biology Fund for Excellence). The Tg(lhx1a-EGFP) transgenic line was provided by Dr. Neil Hukriede (University of Pittsburgh).

Materials

Anti-fluorescein antibody	Roche/Sigma-Aldrich	11426338910
Bleaching solution			0.8% KOH, 0.9% H2O2 in PBST
Blocking reagent	Roche/Sigma-Aldrich	11096176001	Use for blocking solution, prepare according to manufacture's instruction
Cell strainer	Fisher Scientific	22-363-549	100 μm
E3 medium			5 mM NaCl, 0.33 mM CaCl2, 0.33 mM MgSO4, 0.17 mM KCl, 0.0001% methylene blue
Eyelash manipulator	Fisher Scientific	NC1083208	Use to manipulate larvae
Fixing solution			4% paraformaldehyde, 1% DMSO in PBS; heat at 65°C while shaking until the powder dissolves, then add DMSO after it cools down
Fluorescein probe synthesis	Roche/Sigma-Aldrich	11685619910
Glass vial	Fisher Scientific	03-338B
Hatchfry encapsulation	Argent
Hyb- solution			50% formamide, 5X SSC, 0.1% Tween-20
Hyb+ solution			HYB-, 5 mg/mL torula RNA, 50 ug/mL heparin
MAB (10X)			1 M maleic acid, 1.5 M NaCl, pH 7.5
MABT			1X MAB, 0.1% Tween-20
Maleic acid	Sigma-Aldrich	M0375
Paraformaldehyde	Sigma Aldrich	158127
PBS (10X)			8% NaCl, 0.2% KCl, 1.44% Na2HPO4, 0.24% KH2PO4
PBST			1X PBS, 0.1% Tween-20
PBST2			1X PBS, 0.2% Tween-20
Powder food			Mix 2 g of each of spirulina and hatchfry encapsulon in 50 mL of fish system water and shake well
Proteinase K	Sigma-Aldrich	P5568	Use to permeabilize larvae
Proteinase K solution			20 μg/mL, 1% DMSO final concentration in PBST
Spirulina microfine powder	Argent
SSC (20X)			3 M NaCl, 0.3 M sodium acetate anhydrous, pH 7, autoclave
SSCT (0.2X)			Dilute from 20X SSC, 0.1% Tween-20
SSCT (2X)			Dilute from 20X SSC, 0.1% Tween-20
Staining buffer			100 mM Tris pH 9.5, 50 mM MgCl2, 100 mM NaCl, 0.1% Tween-20
Staining solution			200 μg/mL iodonitrotetrazolium chloride, 200 μg/mL 5-Bromo-4-chloro-3-indolyl phosphate disodium salt, in staining buffer
Stopping solution			1 mM EDTA, pH 5.5, in PBST
Torula (yeast) RNA	Sigma-Aldrich	R6625
Tricaine	Sigma Aldrich	E10521	2%, pH 7
Wash buffer			50% formamide, 2X SSC, 0.1% Tween-20

References

Kinth, P., Mahesh, G., Panwar, Y. Mapping of zebrafish research: a global outlook. Zebrafish. 10 (4), 510-517 (2013).
Grunwald, D. J., Eisen, J. S. Headwaters of the zebrafish – emergence of a new model vertebrate. Nature Reviews. Genetics. 3 (9), 717-724 (2002).
Wingert, R. A., Davidson, A. J. The zebrafish pronephros: a model to study nephron segmentation. Kidney International. 73 (10), 1120-1127 (2008).
Drummond, I. A. Kidney development and disease in the zebrafish. Journal of the American Society of Nephrology: JASN. 16 (2), 299-304 (2005).
Swanhart, L. M., et al. Zebrafish kidney development: basic science to translational research. Birth defects research. Part C, Embryo Today: Reviews. 93 (2), 141-156 (2011).
Dressler, G. Advances in early kidney specification, development and patterning. Development. 136 (23), 3863-3874 (2009).
Johnson, C. S., Holzemer, N. F., Wingert, R. A. Laser ablation of the zebrafish pronephros to study renal epithelial regeneration. Journal of Visualized Experiments: JoVE. (54), e2845 (2011).
Marra, A. N., et al. Visualizing gene expression during zebrafish pronephros development and regeneration. Methods in Cell Biology. 154, 183-215 (2019).
McMenamin, S. K., Chandless, M. N., Parichy, D. M. Working with zebrafish at postembryonic stages. Methods in Cell Biology. 134, 587-607 (2016).
Diep, C. Q., et al. Development of the zebrafish mesonephros. Genesis. 53 (3-4), 257-269 (2015).
Zhou, W., Boucher, R. C., Bollig, F., Englert, C., Hildebrandt, F. Characterization of mesonephric development and regeneration using transgenic zebrafish. American Journal of Physiology. Renal Physiology. 299 (5), 1040-1047 (2010).
Diep, C. Q., et al. Identification of adult nephron progenitors capable of kidney regeneration in zebrafish. Nature. 470 (7332), 95-100 (2011).
Diep, C. Q., Mikeasky, N., Davidson, A. J., Cartner, S. C. . The Zebrafish in Biomedical Research: Biology, Husbandry, Diseases, and Research Applications. , 145-150 (2020).
Parichy, D., Elizondo, M., Mills, M., Gordon, T., Engeszer, R. Normal table of postembryonic zebrafish development: staging by externally visible anatomy of the living fish. Developmental dynamics: An Official Publication of the American Association of Anatomists. 238 (12), 2975-3015 (2009).
Guo, R., et al. LIM Homeobox 4 (lhx4) regulates retinal neural differentiation and visual function in zebrafish. Science Reports. 11 (1), 1977 (2021).
Vauti, F., Stegemann, L. A., Vogele, V., Koster, R. W. All-age whole mount in situ hybridization to reveal larval and juvenile expression patterns in zebrafish. PloS One. 15 (8), 0237167 (2020).
Parichy, D. M., Turner, J. M., Parker, N. B. Essential role for puma in development of postembryonic neural crest-derived cell lineages in zebrafish. Developmental Biology. 256 (2), 221-241 (2003).
Yang, H., Wanner, I. B., Roper, S. D., Chaudhari, N. An optimized method for in situ hybridization with signal amplification that allows the detection of rare mRNAs. The Journal of Histochemistry & Cytochemistry. 47 (4), 431-445 (1999).
McCampbell, K. K., Springer, K. N., Wingert, R. A. Analysis of nephron composition and function in the adult zebrafish kidney. Journal of Visualized Experiments: JoVE. (90), e51644 (2014).

Play Video

PDF

DOI

DOWNLOAD MATERIALS LIST

Cite This Article

Kasar, S. N., Grandinette, S. A., Semelsberger, S. D., Diep, C. Q. In Situ Hybridization in Zebrafish Larvae and Juveniles during Mesonephros Development. J. Vis. Exp. (174), e62930, doi:10.3791/62930 (2021).

Automatically Generated