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.
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.
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 phenotype3,4,5,6,7. 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 acini8,9,10. 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 plane8,9,10. 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 structures11,12. 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 developed15,16,17,18,19,20. 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 function15,17,19. 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 tubes7,22. 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 spheroids15,20. 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 efficiency21,23. 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.
1. Generation of cysts
NOTE: This protocol can be performed with any type of hydrogel, if the gelation allows embedding of cells.
2. Cyst quantification
3. Cell viability
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.
5. Epithelial polarity assessment by immunofluorescence
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 studies7,8,9,10,15,18,23. The method proposed in this protocol, by recording the whole number of cysts and their respective sizes over the time of the experiment, allows for the analysis of the evolution of cyst formation and growth (Figure 4).
Based on phase contrast images, on day 0, 8 hours after cell seeding mostly small cell aggregates are found embedded into the hydrogel. On day 1, small cysts of median diameter of 42.95 (26.53, 50.47) (first, third quartile) μm and fusion of cysts scattered throughout the hydrogel are noticeable. By day 4, it is common to observe aggregate structures as well as cysts of median diameter of 75 (56.48, 97.97) μm. By days 7 and 10 the median cyst diameter reached 108.67 (75.31, 141.76) μm and 186.46 (113.98, 278.29) μm, respectively (Figure 4A-C). Interestingly, the cyst formation efficiency increases from 70.03 ± 5.05 cysts/1000 cells on day 1 to 99.83 ± 12.81 cysts/1000 cells on day 4 remaining constant till day 10 (Figure 4B), suggesting that cysts form essentially from cell aggregates that are present at the time of the embedding or that form during the next 48h, through cell migration or the fusion of small cell aggregates. With regards to the cyst size evolution, while the mean size follows a slow and regular slope, the size distribution increases widely along the culture time, illustrating that the various cysts do not grow at the same speed. Interestingly, this can be linked to our observation (not shown) that cysts are not evenly distributed in the hydrogel, the biggest cysts lying in the center of the hydrogel volume. Since the increase of the cyst diameter mainly relies on the secretion activity (since the cell division rate is limited in NRC derived cysts), it can be inferred that this activity is highly dependent on the hydrogel properties that are not homogenous in the cell culture volume.
We then confirmed the viability of cells after embedding them into the hydrogel (day 0) and cysts on day 10 using FDA/PI live staining (Figure 5A). FDA is a non-fluorescent molecule that only live cells, through an enzymatic reaction, are able to convert to the green fluorescent compound fluorescein26. PI is a non-permeant molecule for live cells that intercalates in the DNA of necrotic cells27. Interestingly, dead cells that represent less than 3% of the whole cells in the culture volume at day 10, are mostly found outside the cysts, as isolated cells or part of small aggregates. However, we noticed that debris from necrotic cells accumulate in some large cysts at day 10 (Figure 5B). Therefore, for the maintenance of cystic cultures, passaging of cysts is recommended before 10 days in those conditions.
Functional assessment
In physiological conditions, the main function of cholangiocytes is to modify canalicular bile via absorptive and secretory mechanisms of which the MDR channel is a key player28. To assess the functionality of cysts, we incubated day 10 cysts with FDA/Hoechst and observed formation of fluorescein and its secretion from the basal into the apical luminal space (Figure 6A,B). Thus, confirming that NRCs in cysts retain their secretory functions. Moreover, the secretion of fluorescein was inhibited by pre-treatment of cysts with the MDR inhibitor Verapamil (Figure 6C), showing that the accumulation of fluorescence FDA into the lumen was due to the secretion through MDR transporter and not by leaking from the intercellular space.
Assessment of cyst polarity
In order to establish polarization of the NRC cysts, we conducted a series of optimization steps in the immunofluorescence protocol. One main hindering in the examination of epithelial cell polarity in the cysts is the frequent collapse of the organoid architecture during the immunofluorescence process, due to the leakage of the fluid contained in the lumen. To circumvent this problem, each step of the immunofluorescence protocol has been evaluated by testing how various conditions might affect the maintenance of cyst structure. We found that modulating the fixing (formaldehyde (2-4%) + sucrose (5-10%)) or permeabilization conditions (0.1-1% of both Triton X-100 and sucrose) did not have much impact on the cyst architecture. These ranges can be used to strongly fix and gently permeabilize the cholangiocytes (Figure 7A). However, we observed that keeping BSA at 0.1% or less during saturation is a key step in maintaining cyst integrity, as higher concentrations result in cyst retraction and lumen collapse (Figure 7A).
Cholangiocyte functions are dependent on their proper apico-basolateral polarity29. To verify that the NRC cysts self-assemble in hydrogel as polarized structures, we confirmed the apical and basolateral localization of F-actin and E-cadherin, respectively. E-cadherin expression in our cysts also indicates that NRCs maintain their epithelial phenotype in hydrogel (Figure 7B) during at least 10 days.
Figure 1: Experimental workflow of cyst formation and characterization. (A) Hydrogel coating of the chamber slide. (B) Cell embedding in the hydrogel. (C) Microscopy of cyst formation. (D) A 10-day follow up assessment of cyst growth, viability, functionality, and polarization. Please click here to view a larger version of this figure.
Figure 2: Image acquisition method. (A) Workflow of the Z-stack acquisition performed along the hydrogel depth from day 1 to 10: Z-stack acquisition (1) image processing of the Z-stack (2) generation of a minimum intensity projection and cyst quantification (3). (B) Image acquisition software screenshots showing the selection of the objective (1), the adjustment of parameters (2), the automatic saving of images (3), and the Z-stack calibration (4). Please click here to view a larger version of this figure.
Figure 3: Method for the quantification of cyst size and cyst formation efficiency. (A) Image processing layout depicting: Z-stacks to analyze (1), its minimum intensity Z-projection (2), the final Z-projection after background subtraction (3) used for cyst counting and cyst size estimation. (B) Cyst identification on the projection (A3) with a zoom of the projection (4) to show the identification of cysts featured by a dark cell shell enclosing a brighter lumen, which are distinguished by blue lines plotted for diameter measurement vs aggregates with a dark and irregular appearance pointed by red arrows. (C) The formula for calculation of cyst formation efficiency for 1,000 cells. Please click here to view a larger version of this figure.
Figure 4: Cyst formation efficiency and cyst size distribution in the hydrogel. (A) Time-lapse showing representative phase contrast images at days 0, 1, 2, 4, 7, and 10 of the 3D cultures. (B) Plot graph with the kinetics of mean cyst formation efficiency ± SEM (n=3). (C) Box and whisker plot showing the cyst size distribution over the time of culture. Black bars represent the first quartile, the median and the third quartile; lines represent the width of the distribution; black dots represent the minimum and the maximum of the distribution, n=3. Please click here to view a larger version of this figure.
Figure 5: Viability of NRC cysts in the hydrogel. (A) Representative fluorescent live images of cultures at day 0 and at day 10, stained with FDA (green=live) and PI (red=dead). Note that the red fluorescence was mainly associated to single cells. (B) Representative fluorescent live image of a necrotic cyst at day 10, where the dead cells (in red) were seen accumulating in the lumen. Please click here to view a larger version of this figure.
Figure 6: Functionality of NRC cysts in the hydrogel. (A) Representative fluorescent live images of a 10-day cyst where the cell’s layer was revealed by nuclei labeling with Hoechst (blue) and the lumen by the secreted FDA (green). (B) Representative phase contrast/fluorescent live images after a secretion test with FDA, which was shown accumulated in the lumen. (C) After the exposition to Verapamil, an MDR inhibitor, representative phase contrast/fluorescent live images of cysts showing that FDA was retained in the cell’s layer. Please click here to view a larger version of this figure.
Figure 7: Immunofluorescence of NRC cysts in the hydrogel. (A) Optimization of the immunofluorescence protocol with bright field images showing representative cyst shapes at each step of the protocol. From left to right: (Living cyst) a live cyst in complete medium before fixation, (Fixation) a cyst after fixation, (Permeabilization) another cyst after permeabilization, (Saturation) a cyst after the saturation step and (Labeling) a cyst at the immunolabeling step. (B) (1-2): Confocal images of a section through a cyst showing the apical surface marker F-actin (red-orange), the basolateral marker E-cadherin (green) and the nuclei stained with DAPI (blue). (3): 3D reconstitution of a set of cysts with the following labelings: red-orange for F-actin and green for E-cadherin. Please click here to view a larger version of this figure.
Supplementary Figure 1: Opening of a stack. Screenshot captures of the software depicting the procedure to open a Z-stack. Please click here to view a larger version of this figure.
Supplementary Figure 2: Stack duplication. Screenshot captures of the software showing the process to duplicate a Z-stack. Please click here to view a larger version of this figure.
Supplementary Figure 3: Generation of a minimum intensity projection. Screenshot captures of the software illustrating the procedure to create a minimum intensity projection from the duplicated Z-stack. Please click here to view a larger version of this figure.
Supplementary Figure 4: Background removal. Screenshot captures of the software portraying the method to remove the background from the Z-stack projection. Please click here to view a larger version of this figure.
Supplementary Figure 5: Contrast enhancement. Screenshot captures of the software outlining the steps to enhance the contrast of the Z-stack projection. Please click here to view a larger version of this figure.
Supplementary Figure 6: Picture calibration. Screenshot captures of the software delineating the process to calibrate the Z-stack and the Z-stack projection in microns. Please click here to view a larger version of this figure.
Supplementary Figure 7: Cyst counting. Screenshot captures of the software depicting the procedure to count cysts on the Z-stack projection with the straight-line tool. Please click here to view a larger version of this figure.
Supplementary Figure 8: Cyst counting check-up. Screenshot captures of the software outlining the method to compare the number of cysts counted on the Z-stack projection and the Z-stack. Please click here to view a larger version of this figure.
Supplementary Figure 9: ROI saving. Screenshot captures of the software showing how to save the ROI set defined by the countings. Please click here to view a larger version of this figure.
Supplementary Figure 10: Cyst size and number measurements. Screenshot captures of the software detailing how to measure and save cyst size and cyst number from the Z-stack projection and the Z-stack. Please click here to view a larger version of this figure.
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 hydrogels8,9,10,21. However, due to lack of 3D quantitative analysis that allows for comparisons between methods in terms of organoids formation or functionality7,8,9,10,15,18, further standardization for hydrogel or drug screening remains out of reach.
To address these deficiencies, we propose a hydrogel-based, reproducible, and standardized protocol to generate epithelial cell-derived cysts. Here, we exemplified it with the formation of biliary cysts in a basal lamina derived hydrogel, from a referenced cholangiocyte cell line. To unlock the limitation of 3D quantification, cyst formation efficiency is calculated relative to the total number of cells seeded into the hydrogel and cyst growth kinetics is measured across a constant hydrogel volume.
We provide a series of systematic steps to generate and characterize cysts, to allow relevant cyst quantitative analysis. To this aim, special efforts have been made to generate a uniform distribution of cell aggregates at the time of hydrogel embedding and circumvent the heterogeneity of the hydrogel’s structure, which impacts cyst formation by setting the conditions to have a representative sample for cyst counting.
Experimental reproducibility is addressed through critical steps such as, filtering cell suspensions to limit cell aggregate size and pre-coating of the chamber slides prior to cell-hydrogel addition to avoid 2D layer formation when cells contact the surface of the culture vessel. Consistent quantification is solved taking pictures along the Z-axis of the hydrogel with a constant set of parameters across different samples and experiments.
Cyst formation efficiency and cyst growth kinetics are estimated from the total number of cells seeded into the hydrogel. Consequently, an adaptable algorithm for image processing is proposed to segment images for cyst counting and cyst size measurements. The novelty of the method proposed is that the counting and measurements are done on Z-stack projections. After removal of the specific background, the number of images to analyze is restricted, allowing for a considerable gain of time and limiting hard disk’s saturation. Immunofluorescence is a significant tool to analyze 3D cultures at the structural level, in particular polarization, key in proper epithelial cell function4. Thus, we undertook the task to carefully optimize the fixation, permeabilization, and blocking steps of the immunofluorescence part of our protocol; troubleshooting BSA concentration to prevent cyst retraction and further lumen collapse.
Altogether the method proposed opens the pathway to generate a simple, reproducible, and costly-effective protocol, 3D cellular cultures and investigate qualitative and quantitative parameters. Furthermore, this method allows for comparisons between different types of matrices: using the same method with poly(ethylene glycol) (PEG)-derived hydrogels we could demonstrate that lumen formation and growth are critically dependent on the hydrogel stiffness and adhesiveness, respectively21. This protocol is also applicable for comparing formation and function of spheroids derived from different cells, which could participate to the standardization of tissue-specific epithelial spheroid models. However, a limitation is that the optimization of culture conditions such as culture media, initial cell seeding, and the time needed for cyst formation might be required for other cell types. In the bile duct field, this work might contribute to answer questions regarding bile duct organogenesis, as well as molecular pathways of disease, and drug testing. This protocol will also find its limit when applied to high throughput analysis since some steps like cyst counting and imaging processing are not automatized yet, even though we propose macros for semi-automatizing the imaging process that could be further developed for automatization. The limitation to automatic processing in this case is the image background. This is due to heterogeneous structure of natural complex hydrogels such basement membrane type gels, but we believe that automatization might be applied to transparent gels such as PEG-derived hydrogels.
The authors have nothing to disclose.
We thank Dr. Nicholas LaRusso (Mayo Clinic, Rochester, Minnesota, United States), who kindly provided the NRC cell line.
This work received the financial support of both the iLite RHU program (grant ANR-16-RHUS-0005) and the DHU Hepatinov.
We thank Isabelle Garcin and Réseau d’Imagerie Cellulaire Paris Saclay for their support on imaging.
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 |