A Rapid Filter Insert-based 3D Culture System for Primary Prostate Cell Differentiation

Summary

Here, we present a method for the establishment of a rapid in vitro system that supports the three dimensional culturing and subsequent luminal differentiation of primary prostate epithelial cells.

Abstract

Conditionally reprogrammed cells (CRCs) provide a sustainable method for primary cell culture and the ability to develop extensive "living biobanks" of patient derived cell lines. For many types of epithelial cells, various three dimensional (3D) culture approaches have been described that support an improved differentiated state. While CRCs retain their lineage commitment to the tissue from which they are isolated, they fail to express many of the differentiation markers associated with the tissue of origin when grown under normal two dimensional (2D) culture conditions. To enhance the application of patient-derived CRCs for prostate cancer research, a 3D culture format has been defined that enables a rapid (2 weeks total) luminal cell differentiation in both normal and tumor-derived prostate epithelial cells. Herein, a filter insert-based format is described for the culturing and differentiation of both normal and malignant prostate CRCs. A detailed description of the procedures required for cell collection and processing for immunohistochemical and immunofluorescent staining are provided. Collectively the 3D culture format described, combined with the primary CRC lines, provides an important medium- to high- throughput model system for biospecimen-based prostate research.

Introduction

The identification and use of cancer therapies that are personalized to individuals are a primary goal in cancer research. Recently, new approaches have been developed that allow for greater ease in the establishment of primary cell cultures, potentially providing ways of both identifying and testing personalized therapies. For example, the R-spondin-based prostate organoid approach¹ allows for three-dimensional (3D) culturing of normal and metastatic prostate cancer cells in a commercial extracellular matrix (e.g., Matrigel), while the Conditionally Reprogramming of Cells (CRC) method developed at Georgetown^2,3 utilizes more standard 2D culture conditions. Specifically, the combination of a Rho kinase inhibitor (Y-27632) and irradiated J2 murine fibroblast feeder cells lead to the indefinite culturing of keratinocyte CRCs². The CRC methodology is extremely robust, with primary cell lines successfully established and maintained indefinitely from the prostate and many other normal and malignant epithelial tissues³. Importantly, our CRC technology allowed for the rapid identification of the etiological basis for recurrent respiratory papillomatosis in a patient who had failed a number of previous drug treatments. In addition, using normal and tumor-derived CRCs, the successful identification of an FDA approved drug, vorinostat, was made within two weeks of initial tissue biopsy. The patient was placed on vorinostat, resulting in the successful treatment of their disease⁴.

The normal prostate gland is comprised of luminal, basal and the rare neuroendocrine cells⁵. Luminal cells form the columnar epithelial layer of the gland and express the androgen receptor (AR), as well as other luminal markers such as cytokeratins 8 and 18 and prostate-specific antigen (PSA)⁶. Conversely, basal cells are localized beneath the luminal layer and express cytokeratin 5 and p63, but low levels of the AR⁵. We^7,8,9 and others¹⁰ have successfully used prostate CRCs in preclinical mechanistic drug sensitivity investigations. However, when grown under standard 2D tissue culture conditions, these cells fail to fully engage AR signaling¹⁰. Importantly, when placed under the renal capsule of immunodeficient mice, the CRCs regained normal prostate glandular architecture and function indicating that prostate CRCs retain their lineage commitment when placed in a permissive environment. The development of the filter insert-based cell culture system described here allows for the rapid (2 weeks) in vitro differentiation of prostate CRCs as evidenced by the increased expression of the AR and AR target genes as well as decreased levels of p63.

The filter inserts used contain polycarbonate membranes (pore size, 0.4 µm) that can support the culturing of mammalian cells. The system, as developed, makes use of normal and malignant prostate CRCs, 6 well culture dishes and the filter inserts. Cell culture media conditioned by J2 cells¹¹ is placed in the bottom chamber and prostate differentiating media in the top chamber. The techniques described herein support prostate luminal cell differentiation within a 2 week timeframe, consistent with the goals of personalized medicine. It was also imperative to develop the methodologies that allow for the comprehensive molecular, genetic and cellular profiling of the cultures. Approaches for isolating DNA, RNA and protein from cells released from the filter surface have been developed and streamlined for accurate repeat sample processing. Finally, the methodology required for removing the filter to enable embedding, sectioning and for H&E, immunohistochemical and immunofluorescent staining, is fully described.

Protocol

1. Establishment of the 3D Cell Culture Insert System

1. Place 2 polycarbonate cell culture inserts in an inverted orientation (filter side up) down in a 6 well plate (Figure 1A).
2. Apply a thin layer of 0.1% gelatin in water to the bottom side of the insert and allow to dry (10-20 min) in a biological safety cabinet to maintain sterility.
3. Repeat step 1.2 two more times for a total of 3 applications of 0.1% gelatin on the inserts.
   NOTE: The gelatin coating will help limit diffusion between the chambers.
4. To collect the primary CRCs from standard culture conditions, add 5 mL of PBS to wash the culture flask.
   1. Trypsinize the cells using (1 mL for a T-25 and 2 mL for a T-75) 0.25% trypsin-EDTA for 5 min at 37 °C. Gently tap the side of the flask to aid in dislodging the cells. Then proceed to stop the trypsin reaction and collect the cells by adding 5 mL of complete DMEM.
   2. Collect the cells in a 15 mL tube. Centrifuge the tube at 4 °C and 188 x g and count using an automated cell counter or a hemocytometer.
   3. Re-suspend 600,000 CRCs in 250 μL conditioned media (CM) and add to the properly oriented (filter side down) culture insert (Figure 1B). This is referred to as the inner chamber.
      Note: CM is F-media conditioned by irradiated J2 cells and contains 10 μm Y-27632 as previously described^7,8,9,11.
5. Apply 2 mL of CM to the outer chamber of the 6 well plate and incubate at 37 °C overnight (for at least 18 h).
6. Carefully remove the CM on the inner chamber with a 1 mL or 200 μL pipette and slowly add differentiation media (DM) to the inner chamber with a 1 mL pipette until full. Be careful to not disturb the cell layer.

2. Maintenance of 3D Cultures

1. Check the cultures every day. Healthy cells appear as shown in Figure 2.
2. Change the CM in the outer chamber every day or every other day depending on the metabolism of the cells.
3. When the media of the inner chamber changes color (yellow), carefully remove the media on the inner filter chamber with a 1 mL or 200 μL pipette.
4. Aspirate the media in the outer 6 well plate chamber with an aspirating tip.
5. Using a 1 mL pipette, slowly apply fresh DM to the inner chamber until full. Be careful not to scrape or otherwise dislodge the cell layer.
6. Replace the media in the outer chamber with 2 mL of fresh CM.
7. Maintain the cultures for 2 weeks, and then proceed to processing for the desired bimolecular isolation.
   NOTE: Each row in the 6 well plate, a total of six inserts (Figure 1B), should be processed per experiment to acquire enough cells for DNA, RNA or protein for analysis.
8. Aspirate media in the outer chamber and rinse with 2 mL phosphate buffered saline (PBS).
9. Carefully remove media from the inner chamber with a 1 mL or 200 μL pipette and add 500 μL PBS. Avoid scraping or otherwise disturbing the cells on the membrane.
10. Aspirate PBS from the outer chamber and carefully remove PBS from the inner chamber with a 1 mL or 200 μL pipette. Once the PBS has been removed, proceed directly to the appropriate application detailed below. Do not allow the membrane to dry out. The culture can be kept briefly in the PBS until the application is ready to begin.

3. Processing the Filters for Pellet Banking

1. Add 100 μL  0.25% trypsin-EDTA to each inner chamber and incubate for 5 min at 37 °C.
2. Briefly and carefully agitate/scrape the cells on the membrane surface with a 200 μL pipette while pipetting up and down (avoid puncturing the membrane). Incubate for 1 min at 37 °C.
3. Add 250 μL of CM to the first inner chamber and pipette up and down gently to rinse the filter.
4. Transfer resuspended cells to the adjacent filter chamber that contains the same media conditions and repeat pipetting up and down.
5. Repeat this procedure for each of the inserts of a single condition. Collect and transfer cells to a 1.5 mL centrifuge tube.
6. Rinse each inner chamber with an additional 100-200 μL of CM to collect any remaining cells. Add to the 1.5 mL centrifuge tube in step 3.5.
7. Spin the cells at 423 x g in a microcentrifuge at 4 °C for 5 min.
8. Aspirate the supernatant and wash the cell pellet once with 1000 μL PBS.
9. Spin again at 423 x g in a microcentrifuge at 4 °C for 5 min.
10. Aspirate PBS and freeze at -80 °C for later use.

4. Processing the Filters for RNA or DNA Isolation

1. Add 200 μL of guanidinium thiocyanate-phenol-chloroform or similar extraction reagent to the inner chamber and briefly agitate the cells on the membrane surface by pipetting up and down.
2. Incubate in the extraction reagent for 5 min at room temperature with the outer chamber dry.
   1. As the filter may dissociate from the insert, wash the disassociated filter membrane by pipetting the extraction solution up and down. Collect as much of the extraction reagent as possible by tilting the 6 well plate and aspirating any residual liquid.
3. Follow the manufacturer's protocol for purification and recovery of DNA, RNA or protein.

5. Processing the Filters for Protein Isolation

1. Place the filter insert in the 6 well plate on ice. To the inner chamber, add 10 μL of protein lysis buffer supplemented with 1 mM sodium fluoride (NaF), 1 mM sodium vanadate (NaV), 100 mM dithiothreitol (DTT) and 100 μL of anti-protease cocktail.
2. Agitate/scrape the cells on the membrane surface with a 20 μL pipette while pipetting up and down. Avoid generating bubbles in the lysis buffer.
3. Incubate the 6 well plate with filter inserts on ice for 10 min.
4. Repeat scraping and then rinse the membrane surface with the lysis buffer.
5. Collect the lysates from the 6 inserts and transfer to a 1.5 mL centrifuge tube on ice.
6. Rinse the first membrane with an additional 10 μL of lysis buffer and transfer to the next filter.
7. Repeat step 5.6 for all inserts, collecting any residual lysis buffer solution and add to the 1.5 mL tube (step 5.5).
8. Incubate the sample on ice for an additional 5 min.
9. Spin at maximum speed (16,873 x g in a table top centrifuge) for 15 min at 4 °C.
10. Pipette lysate supernatant into a fresh 1.5 mL tube.
11. Proceed to the analysis of protein concentration or store lysates at -80 °C.

6. Processing for H&E and Immuno-staining

1. Add 500 µL and 1 mL of 10% NBF (neutral buffered formalin) to the inner and outer chamber and let incubate overnight at 4 °C.
2. Aspirate the NBF from the outer chamber and add 1 mL hydroxyethyl agarose (HEA) processing gel to a 1.5 mL centrifuge. Slowly melt the agarose in a microwave using low power and repeated 10-20 s pulses until the agarose is melted.
3. Keep the HEA in a 37 °C warm bath to prevent solidification until ready to use.
4. Remove the NBF from the inner chamber and apply 25 μL of molten HEA to the inner chamber and allow the agarose to solidify for 2-5 min.
5. Wet 2 foam histology pads in 10% NBF and place one pad in an embedding cassette (see Figure 3D).
6. Use a #11 blade scalpel (which has a very sharp, fine-pointed blade) to score the filter from the bottom side of the insert chamber, partially releasing it from the plastic insert chamber.
7. Place a small amount (100-200 μL) of NBF in a Petri dish and immerse the partially dislodged filter in the NBF (Figure 3A).
8. With a #10 blade scalpel, gently press against the middle of the filter, from the inside of the insert chamber, to fully dislodge the filter from the insert barrel (Figure 3B). If there is any part of the filter that is still attached to the barrel, sever it with the scalpel.
9. Cut the HEA-coated filter in half with the #10 blade scalpel (Figure 3C).
10. Place each half of the filter onto the foam pad in the histology cassette prepared in step 6.4 (Figure 3D).
11. Add the second 10% NBF soaked sponge to the cassette, sandwiching the filter.
12. Snap seal the cassette, place in NBF, and incubate overnight.
13. Process filters into paraffin blocks for sectioning and staining as described previously¹².

Results

The cell culture insert based system is a relatively simple and rapid procedure for producing 3D cultures of prostate CRCs that supports luminal cell differentiation. A schematic of the system is shown (Figure 1A) highlighting the application of the gelatin coating to the bottom surface of the filter insert. The inserts are only overturned for the application of the gelatin. In Figure 1B the filters are in the appropriate orientation for culturing. Using ...

Discussion

Primary cell lines are an important and rapidly developing platform for cancer research. The culture insert-based 3D culture system supports the differentiation of primary prostate CRCs within a two-week timeframe. The CRC filter method represents a new, medium throughput method for prostate research. Existing mouse PDX models are time consuming and extremely expensive, and many of the PDX samples cannot be grown in culture, limiting investigator-initiated experimentation and their usefulness. In addition, while success ...

Materials

Name	Company	Catalog Number	Comments
Corning Costar Snapwell Culture Inserts	Corning	3801
Millicell Cell Culture Inserts	Millipore	PIHP01250
Multiwell 6 Well	Falcon	353046
Gelatin 0.1% in water	Stemcell Technologies	7903
Sterile Saftey Scapel 10 Blade	Integra Miltex	4-510
Sterile Standard Scalpel 11 Blade	Integra Miltex	4411
RIPA Lysis and Extraction Buffer	Thermofisher Scientific	89900
Sodium Fluoride	Fishcer Scientific	S299-100
Sodium Vanadate	Fishcer Scientific	13721-39-6
Dithiothreitol	Sigma-Aldrich	3483123
Protease Inhibitor Cocktail (AEBSF, Aprotinin, Bestatin, E-64, Leupeptin and Pepstatin A)	Sigma-Aldrich	P8340
0.25% Trypsin-EDTA (1x)	Thermofisher Scientific	25200-056
DMEM	Thermofisher Scientific	11965-092
FBS	Sigma-Aldrich	F2442
Glutamine	Thermofisher Scientific	25030081
Penicillin Streptomycin	Thermofisher Scientific	15140-122
F-12 Nutrient Mix Media	Thermofisher Scientific	11765054
Y-27632 dihydrochloride Rock inhibitor	Enzo	ALX-270-333-M025
Hydrocortisone	Sigma-Aldrich	H0888
EGF	Thermofisher Scientific	PHG0315
Insulin	Thermofisher Scientific	12585-014
Cholera Toxin	Sigma-Aldrich	C3012
Gentamicin	Thermofisher Scientific	15710-064
Fungizone	Fisher Scientific	BP264550
Trizol Reagent	Invitrogen	15596026
Histogel Specimen Processing Gel (hydroxyethyl agarose (HEA))	Thermo Scientific	HG-4000-012
Non-Adherent Dressing	Telfa	KDL2132Z
Cell Culture Dish	Sigma	SIAL0167
HISTOSETTE II Tissue Processing / Embedding Cassettes	Crystalgen	CG-M492