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Method Article

Isolation of Primary Human Proximal Tubule Epithelial Cells and Their Use in Creating a Microphysiological Model of the Renal Proximal Tubule

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DOI:

10.3791/67997

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May 9th, 2025

 ,  ,  ,  ,  , 
1Department of Pharmaceutics, School of Pharmacy, University of Washington, 2Department of Pharmacy, School of Pharmacy, University of Washington, 3Kidney Research Institute, Division of Nephrology, Department of Medicine, University of Washington, 4Barbara T. Murphy Division of Nephrology, Samuel Bronfman Department of Medicine, Icahn School of Medicine at Mount Sinai

* These authors contributed equally

In This Article

Summary

We present an optimized protocol for processing whole human kidneys to isolate and culture primary renal proximal tubule epithelial cells and the application of these cells in a three-dimensional, microfluidic, microphysiological platform to recapitulate the renal proximal tubule.

Abstract

Kidney disease affects over 850 million people globally, including 37 million Americans. Risk factors for chronic kidney disease include environmental influences, genetic predispositions, co-existing medical conditions, and a history of acute kidney injury. These factors often take months or years to develop, complicating longitudinal studies of disease etiology and pathophysiology. Advanced kidney models are needed to improve our understanding of disease mechanisms and enhance nephrotoxicity prediction in drug development. Proximal tubule epithelial cells (PTECs) in the kidney play a critical role in xenobiotic and toxin clearance as well as the reabsorption of essential nutrients. We have previously demonstrated that three-dimensional (3D) microphysiological system (MPS) platforms, populated with isolated primary PTECs, can be used to investigate renal drug interactions, assess nephrotoxicity of compounds, and predict drug clearance. Here, we present protocols for isolating and culturing primary PTECs from whole human kidneys and for seeding them into a 3D MPS platform that mimics in vivo renal physiology. This protocol enables long-term studies supporting PTEC viability, physiological morphology, and functional polarization of key transporter proteins in MPS devices for up to 6 months.

Introduction

The kidney plays a critical role in the clearance and elimination of a wide array of xenobiotics, toxins, and endogenous compounds from the body. This is achieved by filtering blood to remove waste products and by regulating electrolyte balance, fluid levels, and pH. Each human kidney contains around one million nephrons, the structural and functional units of the kidney1. Within these nephrons, specialized epithelial cells in the proximal tubules, known as proximal tubule epithelial cells (PTECs), are responsible for reabsorbing essential molecules such as glucose, amino acids, and ions, as well as for secreting drug substrates and potentially toxic substances into the urine2,3,4. In some cases, PTECs may also reabsorb compounds from the urine back into the bloodstream4. Due to their critical role in drug and toxin interactions, primary PTECs isolated from human kidneys provide a valuable tool for studying renal drug-drug interactions (DDIs) and assessing the nephrotoxicity of compounds.

Drug-induced nephrotoxicity poses a significant clinical challenge, as it can lead to acute kidney injury and chronic kidney disease5. Therefore, a deeper understanding of the renal proximal tubule physiology is essential for accurately predicting and characterizing the nephrotoxic potential of drugs and toxins. Traditional in vitro models, including immortalized renal cell lines (e.g., RPTEC-TERT1, HK-2), have limitations in mimicking the complex structure and function of the human proximal tubules6, which operate under dynamic, laminar flow (with a low Reynolds number) and a uniform extracellular matrix (ECM) in vivo7,8. Additionally, traditional two-dimensional (2D) models often fail to functionally express major renal transporters (e.g., organic anion transporter 1 and 3 (OAT1 and OAT3), organic cation transporter 2 (OCT2)) due to rapid degradation and internalization of these proteins6,9,10,11. Animal models, while informative, may not fully replicate human renal physiology and often lack translatability due to species differences in transporter expression and activity12. For example, mOct1 is basolaterally expressed in mouse PTECs, while in humans, the membrane protein expression of OCT1 in the kidney is undetectable13,14.

Advancements in microphysiological systems (MPS) and organ-on-a-chip technologies have enabled researchers to develop in vitro models that closely mimic the three-dimensional (3D) architecture and dynamic fluid flow conditions of human organs15. Our group has previously characterized two MPS models with PTECs16,17, and has utilized these models to conduct toxicity studies18,19,20 and predict drug disposition accurately21. The use of primary PTECs in these models provides significant advantages due to their ability to retain functional characteristics observed in vivo.

Here, we present the protocols for the isolation of human PTECs from an intact human kidney obtained from a deceased donor via a United Network for Organ Sharing (UNOS)-approved organ procurement organization and applying these cultured human PTECs within an MPS platform.

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Protocol

All work was conducted in compliance with the University of Washington's human tissue handling guidelines. Suitable donors meet the following requirements: less than 36 h of cold ischemic time (CIT), no known history of kidney diseases, dialysis, or any other medical conditions (e.g., diabetes mellitus type 1 or 2, hepatitis B, hepatitis C, human immunodeficiency viruses (HIV), viral/bacterial meningitis, methicillin-resistant Staphylococcus aureus infection, syphilis, sepsis, or Covid-19). The whole human kidneys used in this study were sourced through a UNOS-approved OPO.

1. Biosafety cabinet preparation

  1. Spray the hood down with 70% ethanol. Decontaminate all surfaces and items inside the cabinet to create a sterile environment.
  2. Lay down blue absorbent pads. Perform all tissue work over these pads.
  3. Ensure that necessary equipment is available in the biosafety cabinet and properly sterilized (razor blades, serological pipette tips, serological pipette gun, 100 µm cell strainers, p1000 tips, 1000 µL micropipette, 15 cm circular culture dishes, and conical tubes).

2. Kidney pre-processing preparation

  1. Prepare kidney digestion solution by adding 0.75 mg/mL collagenase IV + 0.75 mg/mL dispase II into Dulbecco's Phosphate Buffered Saline (DPBS) with calcium and magnesium. Filter the solution through a 0.2 µm sterile membrane filter.
    NOTE: For a whole human adult kidney, approximately 14 50-mL conical tubes, each containing ~35 mL of digestion solution (totaling 500 mL), are required.
  2. Prepare PTEC media by adding 4.425 g of Dulbecco's Modified Eagle Medium (DMEM)/F12 powder without glucose, 0.5 g of D-glucose powder, 0.6 g of sodium bicarbonate powder, 5 mL of 100x insulin-transferrin-selenium supplement (containing 1000 mg/L insulin, 550 mg/L transferrin, and 0.67 mg/L sodium selenite), 0.5 mL of 50 µM hydrocortisone, and 5 mL of 100x antibiotic-antimycotic solution (containing 10000 units/mL of penicillin G sodium, 10000 µg/mL streptomycin sulfate, and 25 µg/mL amphotericin B in 0.85% saline) into 500 mL of sterile autoclaved ultrapure (Type 1) water. Filter the media through a 0.2 µm sterile membrane filter. Thaw fetal bovine serum (FBS) and make 10 mL aliquots in 14 50 mL conical tubes.
  3. Gather and label an additional set of 50-mL conical tubes. At this step, ensure there are 3 sets of 14 50 mL tubes.
  4. Pre-warm the orbital shaker to 37 °C.

3. Isolation of PTECs from the whole kidney

  1. Using a sterile technique, place the shipping container with the tissue sample into the biosafety hood. Remove the bag from the box and spray the outside with 70% ethanol before putting it in the hood.
  2. Place the kidney on a round 15-cm culture dish. Aspirate/Discard the remaining media.
  3. Remove the surrounding fat and the renal capsule using sterile razor blades. Gently score the renal capsule to create a slit down the center.
  4. Using tweezers, pull off the capsule and use razor blades to slice off any fat attached to the kidney. Discard both the capsule and fat into another 15 cm culture dish.
  5. Separate the cortex (~1 cm thick) from the medulla. Discard the medulla.
    NOTE: The cortex has a lighter brownish-yellow color compared to the medulla.
  6. Using a razor blade, mince the tissue into <1 cm3 pieces until a slurry-like appearance.
  7. Add a small amount of kidney digestion buffer into the dish and transfer the slurry into the first set of 50 mL tubes containing 35 mL of the kidney digestion solution. Distribute evenly and do not exceed a total volume of 45 mL for each tube.
  8. Transfer all tubes onto the 37 °C orbital shaker and incubate for 30 min at the highest speed that does not cause the tubes to fall out. Transfer the tubes back into the biosafety cabinet after spraying them with 70% ethanol.
  9. Invert the tubes to mix and allow the larger pieces of tissue to settle to the bottom. Transfer as much of the solution as possible to the 50 mL conical tubes containing 10 mL of fetal bovine serum (FBS) without transferring intact tissue. Distribute evenly and do not exceed a total volume of 45 mL for each tube.
  10. Centrifuge the tubes at 200 g for 7 min. Move the tubes back into the biosafety cabinet after spraying them with 70% ethanol.
  11. Carefully aspirate out the supernatant. Add 10 mL of PTEC media into each tube and resuspend the pellets.
  12. Strain the resulting cell suspensions through 100 µm cell strainers into new 50-mL conical tubes.
  13. Centrifuge the resulting cell filtrates at 400 g for 5 min. Move the tubes back into the biosafety cabinet after spraying them with 70% ethanol.
  14. Wash the pellets with 5 mL of DPBS. Resuspend pellets using a p1000 tip.
  15. Centrifuge the tubes at 400 g for 5 min. Move the tubes back into the biosafety cabinet after spraying them with 70% ethanol, then aspirate off the supernatants.
  16. Repeat step 3.15 two more times for a total of three washes. Then, resuspend cell pellets with 15 mL of PTEC media and plate the cells on sterile cell culture T-75 flasks.
  17. Label the flasks appropriately and allow the cells to grow in a sterile incubator at 37 °C and 5% CO2. Allow PTECs to grow undisturbed in the incubator for 48 h before the first media change.

4. Media changes

  1. Aspirate media from the flasks.
  2. Wash cells with 5 mL of pre-warmed DPBS.
  3. Add 5 mL of pre-warmed PTEC media to the T-25 flasks.
  4. Return the flask to the incubator.
  5. Change the media every 48 h until the flask reaches at least 70% confluency for passaging or use in experiments.

5. Passaging PTECs

  1. Aspirate media from the flask. Add 5 mL of pre-warmed 0.05% Trypsin-EDTA into each T-25 flask and incubate at 37 °C for 1 to 2 min to allow trypsin digestion.
  2. Once cells are detached, neutralize trypsin with 5 mL of pre-warmed defined trypsin inhibitor solution.
  3. Resuspend 5 times to dislodge any cells still attached to the flask. Then, transfer cell suspension to 15 mL conical tubes and centrifuge at 400 g for 5 min.
  4. Aspirate out the supernatant.
    NOTE: Stop here to cryopreserve PTECs and move to that protocol.
  5. Resuspend cell pellets with 14 mL of PTEC media per tube. Transfer the cell suspensions to T-75 flasks (1 tube per flask).
  6. Perform a T-shake to distribute cells across the flask evenly. Monitor cells and change the media every 48 h.

6. Cryopreserving PTECs

  1. After step 5.6., resuspend the cell pellets in 2 mL of 10% DMSO and 90% low glucose PTEC media for each 15 mL conical tube, and transfer 1 mL into one cryovial.
  2. Transfer the cryovials to a cell freezing container that allows for temperature-controlled freezing and place the container in a -80 °C freezer for 24 h. After 24 h at -80 °C, transfer cryovials to a liquid nitrogen tank for long-term storage.

7. Thawing PTECs

  1. Thaw the vial from -80 °C in the 37 °C water bath. Do not thaw at room temperature (RT). Once the vial has been partially thawed (there should be a small piece of ice visible), add 1 mL of cell suspension to a 15 mL conical tube with 10 mL of pre-warmed PTEC media.
  2. Spin down the cell suspension at 400 g for 5 min. Aspirate the supernatant and resuspend cells in 5 mL of pre-warmed low-glucose PTEC media.
  3. Transfer the 5 mL cell suspension into a T-25 flask and perform a T-shake to distribute cells across the flask evenly. From here, follow section 4 for media changes.

8. Coating the MPS device with Type I Collagen matrix

  1. Aspirate the PBS from the MPS device and remove the device from the package. Wipe the device dry with medical wipes and label it as desired.
  2. Place the MPS device in a 15-cm circular culture dish and place it in 4 °C until ready for use. Keep medical wipes on the bottom of the dish to prevent moisture on the MPS device.
  3. Keep 1 mL syringes with 22 G Luer-Lok needle blunts attached at -20 °C until use for collagen I injection.
  4. For every four MPS devices that need to be filled, keep one 15-mL conical tube on ice. Use one 1-mL syringe with the needle blunt attached for every 15-mL conical tube.
  5. Using a sterile technique in a biosafety cabinet, open all the ports on the MPS device. Make sure the slits at the top of each screw valve align vertically with the port.
  6. Using a 1 mL syringe/needle blunt assembly, flush the ECM chamber with 1 mL of ethanol into Ports #1, #3, and #6. Aspirate out the ethanol and allow it to evaporate completely (at least 30 s) so it does not penetrate the MPS device from Ports #2, #4, and #5.
  7. Place the MPS device back at 4 °C, and keep PTEC media, M199, and 1 N NaOH on ice.
  8. Calculate the matrix composition for 1 mL of the Type I collagen mixture for approximately four MPS devices according to Table 1 (scale as needed). In the biosafety cabinet, mix PTEC media, M199, and 1 N NaOH in this order, according to the above calculations, and keep all the tubes on ice.
  9. Carefully add the Type I collagen stock with a 1 mL syringe to the premade mix. Mix the collagen mixture by pipetting up and down until the mixture has a stable salmon orange-pink color.
  10. Briefly centrifuge the tube to collect the solution at the bottom. Ensure that there are no bubbles in the solution.
  11. Place the pre-chilled 1 mL syringes with 22 G Luer-Lok needle blunts and the MPS device into the biosafety cabinet and on ice. Fill the pre-chilled 1 mL syringe with the collagen mixture and avoid bubbles completely.
  12. Very slowly and gently inject the collagen solution into Ports #1, #3, and #6 of the chilled device chambers. Hold the device vertically with ports facing down to allow air bubbles to flow up and out of Ports #2, #4, and #5.
    NOTE: There should be a droplet of the collagen mixture at Ports #2, #4, and #5, which indicates that the chambers are fully coated.
  13. Remove the syringe and place it back in the 15 mL tube on ice. Turn the screw valve for Ports #2, #4, and #5 to seal the filled chip and place the chip on the culture dish at 4 °C for 30 min.
  14. After 30 min, transfer the chip with the dish into the biosafety cabinet in a sterile manner and spread the chips out evenly and individually so they warm up uniformly.
  15. Put a moistened medical wipe into each dish (to prevent the collagen I matrix from drying out and peeling away from the MPS device walls) and seal the dishes with a semi-transparent flexible sealing film. Allow the collagen to polymerize overnight at RT.

9. Creating a tubular lumen with Type IV Collagen as the ECM in an MPS device

  1. Sterilize C-flex tubing by flushing the tubes with ultrapure (Type 1) water and pure ethanol, then autoclave the whole line of tubing.
  2. In the biosafety cabinet, open all the ports of the Type I collagen-filled MPS device (the screw valve will be vertical with the ports) and remove the wire protruding from Ports #1, #3, and #6 to form the tubular lumens.
  3. Insert the metal couplers into Ports #1, #3, and #6.
  4. Prepare a 10 mL solution of 5 µg/mL Type IV collagen in PTEC media.
  5. Insert 24 inches of sterile C-flex tubing onto the metal blunts protruding from Ports #1, #3, and #6.
  6. Fill 1 mL syringes fitted with a 22-G Luer-Lok needle blunt with 0.5 mL of Type IV collagen solution.
  7. Place the filled syringe on a syringe infusion pump and connect the tubing from Port #1 to the syringe. Repeat this step for Ports #3 and #6.
  8. Using the syringe pump, deliver the Type IV collagen solution into the MPS ports at a rate of 10 µL/min for 30 min. Once the ports have been infused, allow the collagen to solidify in a 37 °C incubator overnight before using them the next day.
    NOTE: Type IV collagen-coated MPS devices can be stored for up to 1 week at 4 °C.

10. Seeding primary PTECs in an MPS device

  1. Inspect the MPS device under the microscope to ensure the lumen has formed correctly.
  2. Place a pre-sterilized 5 mL syringe with a 22 G needle into a 15 mL tube containing 5 mL of ethanol.
  3. Obtain a PTEC cell pellet in a 15-mL conical tube from a T-25 flask by following steps 5.1. to 5.3. Add 80 µL of PTEC media to the cell pellet and gently resuspend.
  4. Transfer the cell suspension to a 1.5 mL microtube.
  5. Remove the dish containing the MPS device from the incubator and place it in the biosafety cabinet. Close Ports #2, #4, and #5, and turn the screw valve horizontally to the ports.
  6. Gently flick the PTEC-containing tube to resuspend the cells. Fill the syringe with cells and insert the needle into the injection port that is farthest from the ports of the screw valves.
  7. Carefully push down on the plunger of the syringe to inject the cells. Visualize the cells after injection under a microscope.
    NOTE: Cells should be moving through the lumen. If no cells are observed in the lumen, check if the needle has been securely inserted into the injection port and reinsert the needle if needed. A full syringe of cells can fill all three lumens on the device.
  8. Continue cell injections with the other two ports. After the injections, close Ports #2, #4, and #5 and place the MPS device back into the 37 °C incubator. Keep the plate level so the cells do not move out of the lumen by gravity.
  9. For additional MPS devices, wash the syringe with ethanol after it is emptied and wash with DPBS before drawing up cells.
  10. Allow the MPS devices to sit overnight undisturbed.
  11. On the next day, connect the MPS devices to the syringe pumps.
  12. In the biosafety cabinet, fill 5 mL syringes with PTEC media. Then, fit 22 G Luer-Lok tip blunts with the 24-inch section of C-flex tubing attached to the syringes.
  13. Place the PTEC media-loaded syringes into the syringe pump. Prime the lines to remove any air bubbles.
  14. Attach the primed tubing lines to Ports #1, #3, and #6 and turn the screw valves to a vertical position to introduce media flow.
  15. Set the syringe pump flow rate at 0.5 µL/min. Place the dish with the MPS device back into the 37 °C incubator and allow the cells to form tubules (within 5 to 7 days) under continuous media perfusion before starting an experiment.

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Results

Morphology and confluency of isolated primary PTECs over time in 2D culture
Following isolation from the kidney cortex, PTECs were allowed to grow undisturbed for at least 48 h before the first media change. Approximately a week after culturing the cells, small batches of PTECs should appear throughout the culture flask with a uniform epithelial, cobblestone-like morphology (Figure 1A,B). Depending on the growth rates of PTECs from different donors, cell...

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Discussion

MPS, or organ-on-a-chip technologies, offer a highly relevant in vitro platform to recapitulate key aspects of human physiology, thereby reducing the reliance on animal models in drug development and toxicological assessments. Recently, the FDA Modernization Act 2.0 (2022) has allowed the inclusion of MPS, among other alternatives, in Investigational New Drug applications29. This protocol details a standard operating procedure for the dissociation of PTECs from human donor cortical tissue...

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Disclosures

The authors declare that they have no conflicts of interest or financial disclosures relevant to this study.

Acknowledgements

Portions of this work were supported by the NASA contract 80ARC023CA001, the National Center for Advancing Translational Sciences (NCATS) (U2CTR004867, UH3TR000504, UG3TR002158), jointly by the NCATS and the Center for the Advancement of Science in Space (CASIS) (UG3TR002178), the National Institute of Environmental Health Sciences (NIEHS) (P30ES00703), The National Institute of General Medical Sciences (T32GM007750), an unrestricted gift from Northwest Kidney Centers to the Kidney Research Institute, and the School of Pharmacy at the University of Washington (Ji-Ping Wang Award and Bradley Fellowship).

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Materials

List of materials used in this article
NameCompanyCatalog NumberComments
1 mL Luer-Lok Tip SyringesBecton, Dickinson309628
1.5 mL microcentrifuge tubesCELLTREAT Scientific Products229442
15 mL sterile conical polypropylene tubeFisher Scientific14-959-53A
3D microphysiological DeviceNortisTCC-001
5 mL Luer-Lok Tip SyringesBecton, Dickinson309646
50 mL sterile conical polypropylene tubeFisher Scientific12-565-271
Antibiotic-Antimycotic (100x)ThermoFisher Scientific15240062
Collagenase, Type IV, powderThermoFisher Scientific17104019
D-(+)-GlucoseMilliporeSigmaG8270
Defined Trypsin InhibitorThermoFisher ScientificR007100
Dimethyl sulfoxide, Bioreagent, Thermo Scientific ChemicalsThermoFisher ScientificJ66650-AK
Dispase II, powderThermoFisher Scientific17105041
Dulbecco’s MEM (DMEM)/F-12 w/o GlucoseUS Biological Life SciencesD9807-02
Dulbecco's Phosphate Buffered Saline (DPBS), calcium, magnesiumThermoFisher Scientific14040117
Fetal Bovine Serum (FBS), PremiumThermoFisher ScientificA5670701
Finnpipette F2 Good Laboratory Pipetting (GLP) KitsThermoFisher Scientific05-719-511Micropipettes
Fisherbrand SureOne Micropoint Pipette Tips, Universal Fit, Non-FilteredFisher Scientific02707407, 02707410, 02707438
Fresh whole human kidneyNovabiosishttps://www.novabiosis.com/research-organ-allocation-services/Human kidneys were obtained through Novabiosis, a UNOS-approved OPO
Humidified incubator (37 °C and 5% CO2)Fisher Scientific51033556
HydrocortisoneMilliporeSigmaH0888
Incubating Orbital ShakerAvantor12620-946
Insulin-Transferrin-Selenium (100X) (ITS -G)ThermoFisher Scientific41400045
Internal Thread Cryogenic VialsCorning430487
Kimtech Science KimwipesKimberly-Clark Professional34120
Luer Stubs (Blunt needle), 22 G x 0.5 inchesInstech Laboratories, Inc.LS22
Medium 199, Earle's Salts (10x)ThermoFisher Scientific21180021
Megafuge 8 Small Benchtop CentrifugeThermoFisher Scientific75007210
Metal Coupler (blunt)Instech Laboratories, Inc.SC 20/15
Mr. Frosty Freezing ContainerThermoFisher Scientific5100-0036
Nikon Eclipse Ti-S MicroscopeNikon Instrumentshttps://www.thelabworldgroup.com/product/nikon-eclipse-ti-fluorescent-microscope/Original model discontinued 
Nunc Non-treated Flasks, T-25ThermoFisher Scientific169900
Nunc Non-treated Flasks, T-75ThermoFisher Scientific156800
Pipette, 10 mL, Graduated, 1/10 mL, SterileGreiner Bio-One607180
Silicon tubing, C-flex tubing, (ID: 0.020", OD: 0.083")Cole-Parmer06422-00
Single edge razor blade (sterile)BiosealKI-205/50
Sodium BicarbonateMilliporeSigmaS6297
Sodium HydroxideMilliporeSigmaS8045
Sterile Disposable Filter Units with PES MembranesThermoFisher Scientific567-0020
Tissue Culture Treated Dishes, 150 mm  x 20 mm VentedGenesee Scientific25-203
Trypsin-EDTA (0.05%), phenol redThermoFisher Scientific25300054
Type I collagen, rat tailCorning354236
Type IV Collagen, MouseCorning354233

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Proximal Tubule CellsRenal Microphysiological ModelKidney Cell IsolationPrimary Epithelial Cells3D MPS PlatformNephrotoxicity PredictionDrug Transport AssessmentCell Culture TechniquesTrypsin DigestionCell Cryopreservation
Isolation of Primary Human Proximal Tubule Epithelial Cells and Their Use in Creating a Microphysiological Model of the Renal Proximal Tubule
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