Generation and Quantitative Characterization of Functional and Polarized Biliary Epithelial Cysts

Summary

Three-dimensional (3D) cellular systems are relevant models for investigating organogenesis. A hydrogel-based method for biliary cysts production and their characterization is proposed. This protocol unravels the barriers of 3D characterization, with a straightforward and reliable method to assess cyst formation efficiency, sizes, and to test their functionality.

Abstract

Cholangiocytes, the epithelial cells that line up the bile ducts in the liver, oversee bile formation and modification. In the last twenty years, in the context of liver diseases, 3-dimensional (3D) models based on cholangiocytes have emerged such as cysts, spheroids, or tube-like structures to mimic tissue topology for organogenesis, disease modeling, and drug screening studies. These structures have been mainly obtained by embedding cholangiocytes in a hydrogel. The main purpose was to study self-organization by addressing epithelial polarity, functional, and morphological properties. However, very few studies focus on cyst formation efficiency. When this is the case, the efficiency is often quantified from images of a single plane. Functional assays and structural analysis are performed without representing the potential heterogeneity of cyst distribution arising from hydrogel polymerization heterogeneities and side effects. Therefore, the quantitative analysis, when done, cannot be used for comparison from one article to another. Moreover, this methodology does not allow comparisons of 3D growth potential of different matrices and cell types. Additionally, there is no mention of the experimental troubleshooting for immunostaining cysts. In this article, we provide a reliable and universal method to show that the initial cell distribution is related to the heterogeneous vertical distribution of cyst formation. Cholangiocyte cells embedded in hydrogel are followed with Z-stacks analysis along the hydrogel depth over the time course of 10 days. With this method, a robust kinetics of cyst formation efficiency and growth is obtained. We also present methods to evaluate cyst polarity and secretory function. Finally, additional tips for optimizing immunostaining protocols are provided in order to limit cyst collapse for imaging. This approach can be applied to other 3D cell culture studies, thus opening the possibilities to compare one system to another.

Introduction

In the last three decades, the field of in vitro research has advanced towards 3D culture systems. A number of protocols have emerged for culturing cells in 3D as spheroids or aggregates in the presence or absence of a scaffold/matrix, in a drop, in agitation, in microfluidic devices, or floating¹. The use of 3D culture methods has proved its advantages over 2-dimensional (2D) cultures, particularly for epithelial cells, which were shown to self-organize in 3D structures, called cysts or acini. In this case, the cells form a monolayer encircling a lumen, where cells acquire their full epithelial phenotype with improved physiological specific functions².

Numerous studies have contributed to the development of methods for forming these epithelial organoids in natural matrices. This has allowed to recapitulate in vivo cell-cell and cell-microenvironment interactions, to get the establishment and the stability of the epithelial phenotype^3,4,5,6,7. Recently, and in particular with the aim of developing transplantable organoids and deciphering the requirement of the microenvironment for orchestrating the epithelial program, synthetic hydrogels have been developed to enhance the formation of epithelial acini^8,9,10. Unfortunately, these studies report on qualitative data, or present calculation methods using internal references such as the ratio of cysts over non-cysts in a 2D plane^8,9,10. This precludes any comparison between different studies in terms of efficiency, stability, or morphological and physiological characterization of the epithelial organoids.

Microencapsulation of epithelial cells in beads using microfluidic devices has allowed for more realistic quantitative and comparative results. Using this technology, organoids from various cell types were formed and differentiated based on the morphology among different 3D cellular structures^11,12. However, this technology is not easy to work with and requires the use of clean rooms to produce the microfluidic devices. This technology has been established for a few types of hydrogels but requires technical adaptation to be applied to other hydrogels, restricting its versatility. Therefore, most studies intended to develop epithelial organoids rely on the embedding of epithelial cells in a hydrogel bulk. In these methods, the high heterogeneity of gel structuration and cell distribution inside the whole 3D culture is often neglected. Therefore, most of the analyses relate to single 2D images, which represent only very roughly the distribution of the various cellular objects in the whole 3D volume.

Diseases that affect bile ducts, such as cholangiocarcinoma, biliary atresia, primary sclerosing cholangitis, among others, are a major cause of mortality and morbidity. Except for liver transplantation, there are no effective treatments for these conditions¹³. Efforts to investigate bile duct formation, disease causes, and progression will allow the development of novel therapies¹⁴.

Biliary organotypic models of cysts, spheroids or tube-like structures using normal or patient-derived, differentiated, or progenitor-derived cholangiocyte cell lines have been developed^{15,16,17,18,19,20}. Various studies have recapitulated cholangiocyte polarity, expression of cholangiocyte markers, presence of cilia, cholangiocyte secretory and reabsorptive ability, and lumen formation and obstruction; all of which represent important characteristics of cholangiocyte phenotype, morphology, and function^15,17,19. Others have reported maintenance of patient-derived biliary organoids for long periods of time²⁰. Recently, we investigated the role of biochemical and biophysical cues on biliary cysts organogenesis²¹. Importantly, the pathogenesis of biliary atresia was studied in biliary spheroids and tubes^7,22. Furthermore, key features of primary sclerosing cholangitis such as cholangiocyte senescence, secretion of pro-inflammatory cytokines, as well as macrophage recruitment were successfully studied using biliary spheroids^15,20. However, reproducible in vitro 3D quantitative models that physiologically modulate cholangiocyte phenotype, physiology, and microenvironment where these questions can be addressed are still needed. Moreover, only few publications have reported cyst formation efficiency^21,23. This is an important point to establish, particularly when investigating organogenesis, disease cause, and correlation of drug responses with cholangiocyte function and polarization. In addition, with differences in scaffold/matrix used from protocol to protocol, it is difficult to compare between systems. To solve these issues, we propose a quantitative, reliable, and universal method to generate biliary cysts mimicking lumen formation, cholangiocyte polarization, and cholangiocyte secretory function. Importantly, we present a systematic analysis performed along the Z-axis across the 3D gel when evaluating over time, cyst formation efficiency, size, viability, polarization, and functionality. Furthermore, we used a natural hydrogel and normal rat cholangiocytes (NRC)s, as an example for the protocol, but other natural or synthetic hydrogels, as well as epithelial cells could be used for the formation of 3D cystic structures.

Protocol

1. Generation of cysts

NOTE: This protocol can be performed with any type of hydrogel, if the gelation allows embedding of cells.

1. Hydrogel coating
   NOTE: Proper hydrogel coating of the chamber slide is a critical step to avoid the formation of 2D cell layers on the bottom of the well, that might interfere with subsequent cyst imaging and impair the calculation of cyst formation efficiency.
   1. To ensure homogeneity of the gel solution, thaw the hydrogel at 4 °C overnight (O/N).
   2. Precool pipette tips on ice or O/N at -20 °C and an 8-well chamber slide at -20 °C O/N.
   3. Place the hydrogel and the 8-well chamber slide on an ice bucket filled with ice.
   4. In a 15 mL conical tube, prepare a solution containing 40% hydrogel (V/V) in cold NRC complete medium (see Table of Materials) and place the tube on ice.
   5. To coat a chamber slide, using cold pipette tips, add 50 μL of hydrogel solution on the center of each well, and spread over the whole surface using a pipette tip, while holding the chamber slide on ice (Figure 1A).
      NOTE: Spread the hydrogel solution as evenly as possible avoiding bubbles.
   6. To polymerize the hydrogel, incubate the chamber slide for at least 15 min at 37 °C, 5% CO₂.
2. Cell preparation
   1. Warm up NRC complete medium, phosphate buffered saline (PBS), and trypsin-ethylenediamine tetraacetic acid (trypsin-EDTA) in a water bath pre-heated to 37 °C.
   2. While the hydrogel is polymerizing, ensure that NRCs are grown to 70% confluency in a T-25 cm² collagen-coated flask²¹. Wash the cells once with pre-heated 1x PBS.  
   3. Incubate the NRCs with 5 mL of pre-heated 1x PBS (for a T-25 cm² flask) for 20 min at 37 °C, 5% CO₂.
      NOTE: This step, which shortens the incubation time with trypsin-EDTA is instrumental in retaining the self-organizing properties of cells.
   4. Discard the PBS, add 1 mL of trypsin-EDTA, and incubate for 5-10 min at 37 °C, 5% CO₂.
   5. Neutralize with 4 mL of pre-heated complete NRC medium. Collect and transfer the cell suspension into a 15 mL conical tube, and spin at 150 x g for 4 min.
   6. Discard the medium and resuspend the cell pellet in 5 mL of pre-heated medium.
   7. Using a 40 μm cell strainer, filter the cell solution into a 50 mL conical tube and count the cells.
      NOTE: Passing the cells through a strainer is a critical step for the quantitative results to be reproducible i.e., to get almost similar size of cell aggregates to be embedded.
3. Embedding of cell suspension in hydrogel solution
   1. Prepare a solution of 1,600 µL of 80% hydrogel (V/V) in cold complete NRC medium (tube 1); keep in ice. Dilute 5 x 10⁵ cells/mL in 1,600 µL of cold complete NRC medium (tube 2) and keep in ice.
      NOTE: This step must be performed quickly to avoid polymerization of the hydrogel while mixing it with the cell suspension and to maintain cell viability.
   2. To prepare a cell seeding solution of 2.5 x 10⁵ cells/mL in 40% hydrogel (V/V), mix tube 1 and tube 2. Add 400 μL of the cell solution into each well of the hydrogel-coated chamber slide avoiding bubbles (Figure 1B).
   3. Keep the chamber slide in an incubator at 37 °C with 5% CO₂ until media change.
   4. After 2 days in culture, remove 250 μL of the medium from a corner of each well, be careful to not pipette out the hydrogel. Then, slowly add 250 μL of the culture medium. Change the medium every 2 days.
      NOTE: Minimize the movement of the chamber slide, particularly during the cyst initiation.

2. Cyst quantification

1. Cyst imaging
   NOTE: This section should be performed quickly to not compromise the cell viability if the microscope is not equipped with a heating chamber to control CO₂ and temperature. In order to ensure consistent quantification, representative of the cyst distribution in the full hydrogel volume, cysts are imaged via phase-contrast microscopy and serial imaging (Z-stacks), with pre-defined parameters throughout different time points.
   1. Take a Z-stack along the depth of the hydrogel for each time point (Figure 1C, D). In this example, Z-stacks are taken at days 1, 2, 4, 7, and 10.
      NOTE: Check that the initial cell distribution is uniform in the hydrogel to ensure the applicability of this method.
      1. With a phase-contrast microscope equipped with an image acquisition software, select the 10x objective magnification in the manual nose-piece pad window (Figure 2B(1)).
      2. Switch on the white lamp and select the brightfield imaging option.
      3. Switch the camera on by selecting the “Play” button in the bar submenu. Focus on a field of cysts and set the exposure time (Figure 2B(2)). Open the Auto Capture Folder window for an automatic saving of images (Figure 2B(3)).
      4. Open the capture Z-series window and define with the Z screw the top and bottom planes of the Z-stack (same XY coordinates but different Z screened). Adjust the Z-step depending on the objective, the level of resolution and press the button “Run now” to launch the acquisition (Figure 2B(4)).
         NOTE: In this example, cysts are spread over a hydrogel thickness of 520 µm. 26 images are acquired along the hydrogel depth with a 20 µm Z-step interval. Depending on the objective, the Z-step should be adjusted to not miss any cyst and to ensure the detection of single cells and aggregates.
      5. Take at least 3 non-overlapping Z-stacks per well.
         NOTE: This sampling is necessary when, like in this example, cysts are more numerous in the depth of the gel than on the edges due to heterogeneities in the hydrogel polymerization.
      6. In order to have a representative dataset repeat step 2.1.1.5. for 3 wells in total.
         NOTE: The heterogeneous distribution of cysts depends on the type of hydrogel, its polymerization, and the cell line. Considering three Z-stacks per well and three wells per experiment, a minimum of 200 cysts are imaged over nine Z-stacks to characterize cyst formation and cyst growth at each time point.
2. Image processing
   NOTE: In a hydrogel, NRCs can be found as single cells, cysts or aggregates. Cysts are identified by the presence of a round and thin contrasted cell shell enclosing a lumen, while cell aggregates present an irregular shape and do not have a lumen. Aggregates and single cells have a dense and contrasted appearance (Figure 3B(4)).
   1. Open the Fiji software, open the Z-stack and go to the Fiji menu and click File | Open (Supplementary Figure 1). Select the Z-stack to analyze. If needed, select “Virtual Stack” option and click “Yes” for opening (Figure 3A(1)).
   2. Duplicate the stack via Image | Duplicate. Click on the box “Duplicate stack” and click “OK” (Supplementary Figure 2).
      NOTE: In this example, Z-stacks are in .nd2 file format encoded in 16 bits.
   3. Create a minimum intensity projection from the duplicated stack. Go to the Image menu | Stacks | Z Project. Select Projection type “Min Intensity” and click “OK” (Figure 3A(2)) (Supplementary Figure 3).
   4. Subtract the background from the projection. Go to the Process menu | Subtract Background. Type 500.0 pixels of rolling ball radius and click “light background” to render cysts more contrasted than the background (Figure 3A(3)) (Supplementary Figure 4).
      NOTE: The rolling ball radius defines the size of the region on which background subtraction is operated. This parameter must be set to the size of the largest object to identify.
   5. If contrast enhancement is needed, go to Image menu | Adjust | Brightness/Contrast | Auto | Apply. Fiji will automatically optimize brightness and contrast. In (Figure 3A(3)), the lower and upper gray values were set to 49702 and 65452, respectively (Supplementary Figure 5).
      NOTE: If the projection is not calibrated, go to the Analyze menu | Set scale and type the corresponding calibration µm/pixel ratio (Supplementary Figure 6).
3. Cyst counting and cyst size measurements
   1. To measure the approximate cyst diameter, select the Straight-line tool in the Fiji menu and draw a line across the diameter of each cyst on the final projection (Figure 3B(4)). Add the new region of interest (ROI) created for each cyst to the ROI manager: press the “t” shortcut on the keyboard for faster counting and opening of the ROI manager. Click “Show All” to see the counted cysts (Supplementary Figure 7)
   2. Check that no cyst has been left without counting by superimposing the set ROIs from the projection on the Z-stack. To do so, click on the Z-stack window to select it. In the ROI Manager, click “Show All” and move the cursor along the Z-stack to check that image per image, all cysts have been counted (Supplementary Figure 8).
   3. Once new cysts have been counted and ROIs added on step 2.3.1., select the ROI set and save it via the ROI Manager window by clicking More | Save (Supplementary Figure 9).
   4. Select all ROIs in the ROI Manager and click “Measure” in the ROI Manager to get the size of each cyst. This will open a new window of measurements named “Results” numbering each cyst and its estimated size. Then save in .csv format by clicking on the “Results” window and via the menu: File | Save As (Supplementary Figure 10).
      NOTE: A macro can be created to semi-automatically process stacks, estimate cyst number/sizes from the projections, and store the data for faster counting procedure. To do so, select the tool “Record” in the bar menu, by clicking Plugins | Macros | Record.
4. Quantification of cyst formation efficiency
   1. Count the number of cysts at day Y, on a projection (Y=1, 2, 4, 7 or 10).
   2. To calculate the cyst formation efficiency for 1000 cells at day Y, divide the number of cysts counted at that time point by the number of cells seeded at day 0 inferred from the hydrogel volume and multiply by 1000 (Figure 3C, Figure 4).
      

3. Cell viability

1. Prepare a stock solution of fluorescein diacetate (FDA) at 5 mg/mL by dissolving 5 mg of FDA in 1 mL acetone and store at -20 °C.
2. Prepare a stock solution of propidium iodide (PI) at a concentration of 2 mg/mL in deionized water (dH₂O) and store at 4 °C.
3. Prepare NRC medium without fetal calf serum (FCS).
4. To prepare the FDA/PI staining solution, add 4 μL of FDA stock solution (8 µg/mL final concentration) and 25 μL of PI stock solution (20 µg/mL final concentration) into 2.5 mL of NRC medium without FCS.
5. Remove the medium from the chamber slide, add 250 μL of staining solution into each well and incubate 4-5 min in the dark at 37 °C, 5% CO₂. Pipette out the staining solution carefully and wash once with 250 μL of 1x PBS.
6. Carefully add 250 μL of complete NRC medium to each well and take pictures using an inverted fluorescence microscope with Texas red and fluorescein isothiocyanate (FITC) filters. Live cells will be green and dead cells will be red (Figure 5A).
   NOTE: In order to quantify live/dead cells, take Z-stacks across the hydrogel volume following step 2 and adapt the image processing method for fluorescence.

4. Secretion activity

NOTE: The secretion activity through the apical membrane of the cholangiocytes is assessed by the secretion of fluorescein in the lumen. Its specificity can be evaluated by doing the same test with Verapamil, a multi-drug resistant (MDR) transporter inhibitor²⁴.

1. To prepare a staining solution of Hoechst 33258 at 5 µg/mL, add 0.83 μL of Hoechst stock solution (15 mg/mL stock concentration in dH₂O) in 2.5 mL of NRC medium without FCS.
2. Add 250 μL of Hoechst solution in each well and incubate at 37 °C, 5% CO₂ for 15 min.
3. Remove the Hoechst solution and add 250 µL of FDA solution (8 µg/mL final concentration) in each well. Incubate 4-5 min at 37 °C, 5% CO₂.
   NOTE: As soon as cells are exposed to FDA staining solution, the follow up of fluorescein secretion kinetics might be useful to calibrate the time needed for cysts to secrete. To do so, take pictures every min for 1 h via time-lapse imaging. In this example, the time needed to observe NRC secreting cysts in the hydrogel is about 15-20 min.
4. Take images using an inverted fluorescence microscope 5 min after rinsing with medium without FCS. Use 4′,6-diamidino-2-phenylindole (DAPI) and FITC filters to reveal nuclei labeling and fluorescein accumulation in the lumen (Figure 6A). To quantify the number of secreting cysts, take Z-stacks as in step 2 and adapt the image processing steps to fluorescent images.
   NOTE: For the Verapamil test, precede the previous process (steps 4.3. to 4.4.) by an incubation with Verapamil, according to the following conditions:
5. Prepare a stock solution of 10 mM Verapamil in dimethyl sulfoxide (DMSO). To prepare 10 µM working solution, mix 2.5 μL of Verapamil stock solution with 2.5 mL culture medium without FCS.
6. To assess that the fluorescence in the lumen results from MDR secretion, take another slide and add 250 µL of Verapamil working solution in each well and incubate 20 min at 37° C, 5% CO₂
7. Remove the solution and add 250 µL of FDA solution (8 µg/mL final concentration) into each well. Incubate 4-5 min in the dark at 37 °C, 5% CO₂. Then, wash with 250 μL of 1x PBS, before imaging (Figure 6B, C).

5. Epithelial polarity assessment by immunofluorescence

1. To prepare the fixing solution, mix 4% formaldehyde with 5% sucrose, in 1x PBS, pH 7.4 and incubate in a water bath pre-heated at 37 °C.
2. To fix the cells, gently pipette out the culture medium from the well without damaging the matrix. Slowly add 400 µL of the fixing solution to the side of the wells. Incubate for 20 min at room temperature (RT).
   NOTE: Always leave 25 µL of the liquid above the matrix to prevent its damage.
3. Gently remove the fixing solution and wash 3x with 400 μL of 1x PBS at (RT).
4. Pipette out the PBS, add 400 µL of permeabilization solution (0.5% Triton X-100 in 1x PBS) and incubate 10 min at RT.
5. Gently remove the permeabilization solution, followed by 3 quick washes with 400 μL of 1x PBS and a long washing step of 30 min at RT.
   NOTE: At this step, the slide can be stored at 4 °C for 2 days. In this case, seal the slide with a paraffin film to prevent evaporation and matrix drying.
6. Remove the PBS, add 400 µL of blocking solution containing 0.1% bovine serum albumin (BSA) and 10% goat serum in 1x PBS and incubate for 60 min at RT.
   CAUTION: Concentrations of BSA higher than 0.1% will result in lumen retraction and further cyst collapse (see Representative Results section) (Figure 7A).
7. Pipette out the blocking solution and wash once with 400 µL of PBS/0.05% Tween 20 and discard.
8. Add 150 µL of the antibody solution, e.g., E-cadherin antibody diluted 1:400 and Phalloidin 568 (16.2 nM final concentration) in 1x PBS and incubate for 90 min at RT.
   NOTE: This dilution of E-cadherin is the same used as in a standard 2D immunofluorescence protocol.
9. Wash the sample with 400 µL of PBS/0.05% Tween 20, 3x; each time incubating the sample for 10 min at RT.
10. Add 150 µL of the secondary antibody (goat anti-rabbit IgG Alexa Fluor Plus 647), diluted 1:500 in 1x PBS and incubate 60 min at RT.
11. Wash 3x with 400 µL of PBS/0.05% Tween 20, each time incubating the sample for 10 min at RT.
12. Wash 3x with 400 µL of 1x PBS, each time incubating the sample for 10 min at RT.
13. Discard the PBS of the last wash and prepare the chamber slide for visualization via confocal microscopy following one of the two options below.
    1. Add 400 μL of 1x PBS and 50 μL of DAPI per well. The samples can be examined through the bottom of the well without the need of mounting with a coverslip (Figure 7B).
    2. Add 100 µL per well of antifade reagent containing DAPI and let the slide drying O/N at RT.

Results

Formation and characterization of cysts
3D cell culture systems are an important tool to study organogenesis and disease modeling²⁵. Unfortunately, most of these methods are qualitative or use internal quantification performed on a single plane by comparing the number of cysts versus non-cysts, in variable and often unspecified volumes, preventing any comparison in terms of cyst formation efficiency between the various studies^7,

Discussion

In order to study organogenesis and maintenance of 3D cellular structures, various tissues have been modelled, using different cellular origins but also different types of extra-cellular matrices including synthetic hydrogels^8,9,10,21. However, due to lack of 3D quantitative analysis that allows for comparisons between methods in terms of organoids formation or functionality^7<...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
10 µl- Pipette Eppendorf Research Plus	Thermo Fisher Scientific	3120000020
100 µl - Pipette Eppendorf Research Plus	Thermo Fisher Scientific	3120000046
1000 µl - Pipette Eppendorf Research Plus	Thermo Fisher Scientific	3120000062
1X PBS	Thermo Fisher Scientific	14190-094
200 µl - Pipette Eppendorf Research Plus	Thermo Fisher Scientific	3120000054
3,3′,5-Triiodo-L-thyronine sodium salt	Sigma-Aldrich	T5516	NRC complete medium final concentration = 3.4 µg/mL
Acetic acid	VWR	20104-298	0.02N final
Aerosol barrier pipettes tips 10 µl (Fisherbrand)	Thermo Fisher Scientific	2707439
Aerosol barrier pipettes tips 1000 µl (Fisherbrand)	Thermo Fisher Scientific	2707404
Aerosol barrier pipettes tips 200 µl (Fisherbrand)	Thermo Fisher Scientific	2707430
Antibiotic Antimicotic Solution (100X)	Sigma-Aldrich	A5955	NRC complete medium final concentration = 1:100 dilution
Bovine pituitary extract	Thermo Fisher Scientific	13028-014	NRC complete medium final concentration = 30 µg/mL
Bovine serum albumin	Sigma-Aldrich	A2153	1:1000 dilution
Chemically Defined Lipid Concentrate (100X)	Thermo Fisher Scientific	11905-031	NRC complete medium final concentration = 1:100 dilution
Collagen high concentration, rat tail	Thermo Fisher Scientific	354249	50 µg/mL final concentration
Dexamethasone	Sigma-Aldrich	D4902	NRC complete medium final concentration = 0.393 µg/mL
DMEM F12	Thermo Fisher Scientific	21331-020	NRC complete medium final concentration = 1X
E-cadherin Rabbit anti-Human, Rat, Polyclonal	Thermo Fisher Scientific	PA5-32178	1:400 dilution
Eclipse TE300 inverted microscope	Nikon		imaging
Ethanolamine	Sigma-Aldrich	E9508	NRC complete medium final concentration = 0.32 mM
Fetal calf serum	Thermo Fisher Scientific	10270-106	NRC complete medium final concentration = 5:100 dilution
Fluoroshield with DAPI (Mounting medium)	Sigma-Aldrich	F6057
Formaldehyde 16% (W/V)	Thermo Fisher Scientific	28906	4% (W/V)
Goat serum	Thermo Fisher Scientific	16210-064	1:10 dilution
Hamamatsu camera (Digital camera C11440 ORCA - flash 4.OLT)	Hamamatsu		imaging
Hoechst 33258	Sigma-Aldrich	B1155	5 µg/mL final concentration
IgG (H+L) Highly Cross-Adsorbed Goat anti-Rabbit, Alexa Fluor Plus 647	Thermo Fisher Scientific	A32733	1:500 dilution
ImageJ version 2.0.0-rc-69/1.52n			Open source image processing software
Insulin-Transferrin-Selenium (100X)	Thermo Fisher Scientific	51300-044	NRC complete medium final concentration = 1:100 dilution
L-Glutamine (100X)	Thermo Fisher Scientific	25030-024	NRC complete medium final concentration = 1:100 dilution
Matrigel GFR (stock concentration 9.7 mg/mL)	Thermo Fisher Scientific	356231	4:10 dilution
NIS Elements software version 4.50.00	Nikon		image acquisition and display
Non-Essential-Amino-Acids-Solution (100X)	Thermo Fisher Scientific	11140-035	NRC complete medium final concentration = 1:100 dilution
Objective Plan Fluor 10X/0.30 Ph1 DL (∞/1.2 WD 15.2)	Nikon
Prolong Gold Antifade Reagent	Thermo Fisher Scientific	P36931
Propidium Iodide (PI)	Sigma-Aldrich	P4170	20 µg/mL final concentration
Rhodamine Phalloidin	Thermo Fisher Scientific	R415	16.2 nM final concentration
Sir-Actin / Verapamil kit	Spirochrome	SC001	10 µM final concentration
Soybean trypsin inhibitor	Thermo Fisher Scientific	17075-029	NRC complete medium final concentration = 50 µg/mL
Sterile cell strainer 40 µm (Fisherbrand)	Thermo Fisher Scientific	22363547
Sterile pipettes 10 mL (Fisherbrand)	Thermo Fisher Scientific	1367811E
Sterile pipettes 5 mL (Fisherbrand)	Thermo Fisher Scientific	1367811D
Sterile tubes 1.5 mL (Fisherbrand)	Thermo Fisher Scientific	11926955
Sterile tubes 15 mL (Fisherbrand)	Thermo Fisher Scientific	7200886
Sterile tubes 50 mL (Fisherbrand)	Thermo Fisher Scientific	553913
Sucrose	Sigma-Aldrich	S0389	5:100 dilution
Tissue culture treated flask 25cm2 (Falcon)	Thermo Fisher Scientific	353108
Triton X-100	Sigma-Aldrich	T8787	5:1000 dilution
Trypsin-EDTA (0.05%) phenol red	Thermo Fisher Scientific	25300-054	1X
Tween-20	Sigma-Aldrich	P1379	5:10000 dilution
Vitamin (100X)	Thermo Fisher Scientific	11120-037	NRC complete medium final concentration = 1:100 dilution
μ-Slide 8 Well ibiTreat, Ibidi	Clinisciences	80826