Nephrotoxin Microinjection in Zebrafish to Model Acute Kidney Injury

Summary

Renal injuries incurred from nephrotoxins, which include drugs ranging from antibiotics to chemotherapeutics, can result in complex disorders whose pathogenesis remains incompletely understood. This protocol demonstrates how zebrafish can be used for disease modeling of these conditions, which can be applied to the identification of renoprotective measures.

Abstract

The kidneys are susceptible to harm from exposure to chemicals they filter from the bloodstream. This can lead to organ injury associated with a rapid decline in renal function and development of the clinical syndrome known as acute kidney injury (AKI). Pharmacological agents used to treat medical circumstances ranging from bacterial infection to cancer, when administered individually or in combination with other drugs, can initiate AKI. Zebrafish are a useful animal model to study the chemical effects on renal function in vivo, as they form an embryonic kidney comprised of nephron functional units that are conserved with higher vertebrates, including humans. Further, zebrafish can be utilized to perform genetic and chemical screens, which provide opportunities to elucidate the cellular and molecular facets of AKI and develop therapeutic strategies such as the identification of nephroprotective molecules. Here, we demonstrate how microinjection into the zebrafish embryo can be utilized as a paradigm for nephrotoxin studies.

Introduction

AKI is an abrupt loss of kidney function that can lead to devastating health consequences¹. AKI is a significant healthcare issue worldwide due to its high incidence of approximately 20% among hospitalized patients, with even higher rates of 30-50% in critical care cases and the elderly, and mortality rates of 50-70%^1-3. Unfortunately, the prevalence of AKI has been increasing and is projected to escalate further over the next decade, due in part to the diversity of factors that can induce AKI, which include post-operative stress, ischemia, and exposure to nephrotoxins such as antibiotics and chemotherapeutic drugs⁴.

AKI involves sudden cellular damage within the kidney, commonly occurring in nephrons, which are the essential functional units, and are comprised of a blood filter and a segmented tubule that drains urine into central collecting ducts¹. When a significant number of nephrons are damaged during AKI, the immediate effects include an interruption in waste clearance from the circulation, and reduced or abrogated fluid flow through nephrons due to obstruction from dead and dying cells¹. Over time, tubular obstruction can lead to degeneration of entire nephrons, which permanently reduces renal function¹. Physiological alterations in the kidney following AKI also involve complex inflammatory events that can lead to chronic scarring¹.

Despite these outcomes, nephrons have some capacity to undergo regeneration after AKI that reconstitutes the tubular epithelium^5,6. While there has been an increasing molecular understanding of nephron regeneration, the mechanisms remain elusive in many regards and necessitate continued investigation⁷. The degree to which AKI results in permanent renal damage also remains unknown. Current research suggests the regenerative potential for the kidney is the highest following less severe cases of AKI, while more pronounced or repeated episodes lead to chronic kidney disease (CKD) and culminate in end stage renal disease (ESRD) that requires life-saving transplantation or dialysis^8,9. Additionally, individuals already suffering from CKD are at an even higher risk of contracting a severe episode of AKI^8,9. Taken together, it is clear that continued basic and clinical research is vital to understand, treat and prevent AKI.

Research with animal models has been instrumental in appreciating the progression of local and environmental alterations that occur during AKI¹⁰. To expand this understanding as well as develop new therapies, the zebrafish animal model has been employed in a variety of ways^11,12. The nephrons of the zebrafish kidney, in both the embryo and adult, display a high degree of conservation with mammals^13-16. Further, nephron epithelial injury in zebrafish resembles the process in higher vertebrates, whereby the local destruction of tubular cells is followed by intratubular proliferation and reestablishment of nephron architecture^17-19. In the embryo, however, extensive tubule damage from the nephrotoxins like cisplatin is associated with lethality^20,21. By comparison, zebrafish adults survive AKI and exhibit substantive regenerative capabilities in the kidney. For example, following exposure to the aminoglycoside antibiotic gentamicin, zebrafish regenerate tubule epithelial damage and grow new nephron units as well^22-24. While these gentamicin-induced AKI studies have provided invaluable information, understanding renal damage from diverse nephrotoxins remains critical to appreciate the effects and response to different types of damage²⁵.

The zebrafish embryo, due to its size, transparency, and genetic tractability, has many benefits for nephrotoxin studies²⁵, where the method of microinjection^20,21 is used to administer the molecule(s) for investigation. Nephrons are formed by 24 hr post fertilization (hpf) and begin to filter blood by approximately 48 hpf^26,27. Thus, the rapid formation and function of the embryonic kidney facilitates experimental analysis. However, the process of microinjection has technical challenges and there can be a steep learning curve to mastering the technique. In this video article, we describe how to perform microinjections and provide troubleshooting tips in order to enhance the rate of successful injections.

Protocol

The procedures for working with zebrafish embryos described in this protocol were approved by the Institutional Animal Care and Use Committee at the University of Notre Dame.

1. Preparation of Solutions

1. Make a 50x stock solution of E3 embryo media by mixing 73.0 g NaCl, 3.15 g KCl, 9.15 g CaCl₂, and 9.95 g MgSO₄ in 5 L of distilled water, and store at RT.
2. For culturing of zebrafish embryos, dilute the 50x stock solution of E3 embryo media stock to a 1x working solution with distilled water, then add 200 μl of 0.05% methylene blue to every 1 L of 1x E3 to act as a fungicide, and store at RT.
3. Make a pigmentation blocking solution of E3 embryo media with 0.003% 1-phenyl-2-thiourea (PTU) by combining 40 ml of the 50x E3 stock with 0.06 mg PTU. Then bring the volume to a total of 2 L with distilled water.
4. Stir the E3/PTU O/N at RT to get the PTU powder into solution. Then store the E3/PTU at RT.
   Note: The E3/PTU has a shelf life of approximately one week, and older solutions will be less effective at blocking pigmentation development in zebrafish larvae.
5. Make an anesthetic solution of 0.2% Tricaine (MS-222) by adding 1 g of Tricaine to 500 ml of distilled water and adjust the pH to 7.2 with 1 M Tris, pH 9.5.
6. Prepare to make a 2% methylcellulose solution for imaging by placing a solution of 1x E3 (no methylene blue), with 1/10^th volume of 0.2% Tricaine added at 4 °C.
   Note: The methylcellulose solution is a thick, clear solution that is used to gently stabilize live embryos for microscopy. After manipulations are performed the embryos can be washed in 1x E3 to dissolve the methylcellulose without injuring the animal and enabling microscopy at subsequent stages in the same specimen.
7. When cooled to 4 °C, stir the 1x E3/Tricaine solution vigorously on a stir plate and gradually add the appropriate amount of methylcellulose powder while continuing to stir vigorously. Gradually add the powder to the solution to prevent the formation of insoluble methylcellulose aggregates.
8. After all the powder is mixed into the 2% methylcellulose/E3/tricaine solution, stir the composite solution in the 4 °C cold room O/N.
   Note: The cold temperature is best for fully dissolving the powder. If the solution is not clear after one night, stir for an additional workday and/or a second O/N.
9. To remove air bubbles from the 2% methylcellulose/E3/tricaine solution, aliquot the mixture into 1.5 ml tubes and spin at high speed (12,000 x g) at 4 °C for 30 min or up to 2 hr.
10. Place the 2% methylcellulose/E3/Tricaine solution at 4 °C for long-term storage.
    Note: Prior to usage, aliquots should be pre-warmed to RT for working with the zebrafish specimens.

2. Preparation of Tools

1. Prepare an embryo manipulator tool, used for positioning embryos for microinjection, by attaching a gel loading tip on the end of a 5" straight dissecting needle, and secure with tape or superglue.
2. Prepare microinjection needles using a needle puller, by first placing a fire polished 10 cm borosilicate glass with filament into the instrument and secure the borosilicate glass by tightening the handles.
3. Pull the borosilicate glass to fashion fine-tapered needles. Use the following settings: heat 540, pull 245, velocity 200, and time 125.
4. Place needles inside a Petri dish, suspending them on a strip of modeling clay to protect the needle tips, and keep the dish covered to prevent dust accumulation.
5. To finish preparing the needle for microinjections, use a razor blade or fine forceps edge to cut the pulled end of the needle to create a sharp angular injection tip with a diameter of approximately 0.05-0.1 mm.
6. To make the microinjection tray, prepare a 1.5% agarose/E3 solution in a 100 ml Erlenmeyer flask and dissolve the agarose by heating the E3 to a boil in a microwave then allow to cool at RT for approximately 10 min.
7. Pour the cooled agarose/E3 solution into a Petri dish to make a foundation with a depth of approximately 0.5 cm. When this has solidified pour a second layer with a depth of approximately 0.3 cm and insert the prefabricated embryo well mold and allow the agarose to solidify at RT.
   Note: When inserting the mold into the top agar/E3 layer, placing the mold into the agar at an angle to decrease the number of air bubbles.
8. When the entire microinjection tray has set, lift the prefabricated embryo well mold out slowly and carefully using a scoopula, then fill the dish with E3 solution and store at 4 °C.

3. Embryo Preparation

1. Set up zebrafish mating tanks by placing dividers into mating chambers and fill with system water.
2. Place one fish on each side of the divider such that each mating chamber contains one female and one male fish, and cover each mating chamber.
3. The next morning, remove the dividers to enable spawning.
4. Check the fish after approximately 30 min, and after returning the adults to the aquarium, collect their embryos by passing the mating tank water through a fine wire-mesh strainer tool.
5. Invert the strainer over a Petri dish and rinse with E3 to collect the embryos.
6. Incubate the embryos at 28.5 °C O/N.
7. When embryos have reached the 24-26 somite stage²⁶, decant most of the E3 media and then dechorionate by adding 100 µl of 50 mg/ml pronase to each dish of embryos and incubating the dish at RT (23 °C) for approximately 15 min.
   Note: It will take approximately 24-25 hr from the time of fertilization for the embryos to reach the 24-26 somite stage if they are collected in the manner described and incubated O/N at 28.5 °C.
8. Fill the dish with E3 and then swirl gently to dislodge the chorions from the embryos.
9. Decant the E3/pronase and rinse the dish with 25 ml of fresh E3. Repeat rinse step to remove all pronase.
10. To block the development of pigmentation, decant the E3 and replace with 25 ml of fresh E3/PTU when the embryos have reached 24 hr post fertilization.
    Note: For experiments spanning several days, replace the E3/PTU solution with fresh media once daily to keep the dish clean.

4. Microinjection of Nephrotoxin Solution

1. On the day of injection, prepare the desired nephrotoxin solution along with the appropriate vehicle control.
2. Vortex or mix gently to insure the drug(s) is/are in solution, checking the sides of the tube and top of the water column.
   Note: Nephrotoxin solutions can be prepared to contain trace amounts of fluorescently conjugated dextran to monitor microinjection efficiency and also assess renal clearance at subsequent time points^20,28.
3. Load a trimmed microinjection needle with ~2-3 µl of the nephrotoxin by threading a fine gel loading tip into the back of the needle and suspend the needle vertically with a piece of tape to allow the solution to fill the trimmed needle tip by gravity.
4. Once the needle tip is full, secure the loaded needle in the micromanipulator.
5. Test the microinjection volume by placing a drop of mineral oil onto a micrometer slide and inject into the oil to evaluate the droplet size. An injection volume of 500 pl has a diameter of 0.1 mm.
6. Remove the dish of embryos from the incubator, and anesthetize by adding approximately 5 ml of 0.2% Tricaine to the embryo dish.
7. To ensure complete anesthetization, gently touch embryo with the tip of the embryo manipulator tool. Lack of movement indicates sufficient anesthetization.
8. After successful anesthetization, transfer embryos to the injection mold with a transfer pipette.
9. Maneuver each embryo into a different well of the mold placing the head in the deepest area of the well such that the trunk rests along the depression and the tail sticks up out of the depression.
10. Insert the filled needle into the micromanipulator and position the needle tip next to an embryo.
11. Gently insert the needle into the tail vessel by moving the joystick forward and depress the foot pedal to deliver the microinjection.
    Note: Successful injection can be gauged by watching the liquid enter circulation. Further, co-injection of the nephrotoxicant with fluorescently conjugated dextran enables the researcher to verify successful injection subsequent to the procedure.
12. Gently pull back on the joystick to remove the needle from the embryo.
13. After injection, transfer the embryos to a clean dish and rinse to remove the Tricaine and replace with fresh E3/PTU.
14. Incubate the embryo to the desired time point to assess morphology, which can be documented by photography in methylcellulose mounting media, or process for experimental analysis as desired.
    Note: Recovery of embryos should be assessed to determine the percentage of individuals with edema, which commonly indicates renal injury.

Results

A microinjection station set up includes a stereomicroscope, micromanipulator and pressure regulator (Figure 1A). Transillumination of the injection plate is preferable to view specimens during this procedure (Figure 1B). Preparation of the injection needle involves pulling the appropriate borosilicate glass, followed by preparing the edge with cutting and finally back-loading the needle. Optimally, the needle tip is beveled rather than blunt (Fig...

Discussion

A diverse number of therapeutic agents have been associated with AKI²⁹. There have been significant research advances in understanding the damage induced by many individual compounds, such as the aminoglycoside gentamicin³⁰ and the widely used chemotherapeutic cisplatin^31,32. Some pathological changes involved in these conditions, however, remain the subject of ongoing study. One emergent challenge remains understanding how multiple drugs adversely affect patients, especially those in hig...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
Sodium Chloride	American Bioanalytical	AB01915
Potassium Chloride	American Bioanalytical	AB01652
Calcium Chloride	American Bioanalytical	AB00366
N-Phenylthiourea (PTU)	Aldrich Chemistry	P7629
Ethyl 3-aminobenzoate (Tricaine)	Fluka Analytical	A5040
Borosilicate glass	Sutter Instruments Co.	BF100-50-10
Flaming/Brown Micropipette puller	Sutter Instruments Co.	Mo. P097
UltraPure Agarose	Invitrogen	15510-027
Magnesium Sulfate	Sigma-Aldrich	M7506
Methylene Blue	Sigma-Aldrich	M9140
Falcon Diposable Petri Dishes, Sterile, Corning:
60 mm x 15 mm	VWR	25373-085
100 mm x 15 mm	VWR	25373-100
(microinjection tray) 150 mm x 15 mm	VWR	25373-187
Low Temperature Incubator	Fischer Scientific	11 690 516DQ
Micro Dissecting Tweezer	Roboz Surgical Instruments Co.	RS-5010
Micrometer	Ted Pella, Inc.	2280-24