Creating Matched In vivo/In vitro Patient-Derived Model Pairs of PDX and PDX-Derived Organoids for Cancer Pharmacology Research

Summary

A method is described to create organoids using patient-derived xenografts (PDX) for in vitro screening, resulting in matched pairs of in vivo/in vitro models. PDX tumors were harvested/processed into small pieces mechanically or enzymatically, followed by the Clevers’ method to grow tumor organoids that were passaged, cryopreserved and characterized against the original PDX.

Abstract

Patient-derived tumor xenografts (PDXs) are considered the most predictive preclinical models, largely believed to be driven by cancer stem cells (CSC) for conventional cancer drug evaluation. A large library of PDXs is reflective of the diversity of patient populations and thus enables population based preclinical trials (“Phase II-like mouse clinical trials”); however, PDX have practical limitations of low throughput, high costs and long duration. Tumor organoids, also being patient-derived CSC-driven models, can be considered as the in vitro equivalent of PDX, overcoming certain PDX limitations for dealing with large libraries of organoids or compounds. This study describes a method to create PDX-derived organoids (PDXO), thus resulting in paired models for in vitro and in vivo pharmacology research. Subcutaneously-transplanted PDX-CR2110 tumors were collected from tumor-bearing mice when the tumors reached 200-800 mm³, per an approved autopsy procedure, followed by removal of the adjacent non-tumor tissues and dissociation into small tumor fragments. The small tumor fragments were washed and passed through a 100 µm cell strainer to remove the debris. Cell clusters were collected and suspended in basement membrane extract (BME) solution and plated in a 6-well plate as a solid droplet with surrounding liquid media for growth in a CO₂ incubator. Organoid growth was monitored twice weekly under light microscopy and recorded by photography, followed by liquid medium change 2 or 3 times a week. The grown organoids were further passaged (7 days later) at a 1:2 ratio by disrupting the BME embedded organoids using mechanical shearing, aided by addition of trypsin and the addition of 10 µM Y-27632. Organoids were cryopreserved in cryo-tubes for long-term storage, after release from BME by centrifugation, and also sampled (e.g., DNA, RNA and FFPE block) for further characterization.

Introduction

Cancers are a collection of diverse genetic and immunological disorders. Successful development of effective treatments is highly dependent on experimental models that effectively predict clinical outcomes. Large libraries of well-characterized patient-derived xenografts (PDXs) have long been viewed as the translational in vivo system of choice to test chemo- and/or targeted therapies due to their ability to recapitulate patient tumor characteristics, heterogeneity and patient drug response¹, thus enabling Phase II-like mouse clinical trials to improve clinical success^2,3. PDXs are generally considered as cancer stem cell diseases, featuring genetic stability, in contrast to cell line derived xenografts². Over the last few decades, large collections of PDXs have been created throughout the world, becoming the workhorse of cancer drug development today. Although widely used and with great translational value, these animal models are intrinsically costly, time consuming and low throughput, therefore inadequate for large scale screening. PDX are also undesirable for immuno-oncology (IO) testing due to an immune-compromised nature⁴. It is thus impractical to take full advantage of the available large library of PDXs.

Recent discoveries, pioneered by the Hans Clevers’ laboratory⁵, have led to the establishment of in vitro cultures of organoids generated from adult stem cells in most human organs of epithelial origin⁵. These protocols have been further refined to allow the growth of organoids from assumed CSCs in human carcinomas of various indications^6,7. These patient-derived organoids (PDOs) are genomically-stable^8,9 and have been shown to be highly predictive of clinical treatment outcomes^10,11,12. In addition, the in vitro nature of PDOs enables high-throughput screening (HTS)¹³, thus potentially offering an advantage over in vivo models and leveraging large organoid libraries as a surrogate of the patient population. PDOs are poised to become an important discovery and translational platform, overcoming the many limitations of PDXs described above.

Both PDO and PDX are patient-derived and CSC-driven models, with the ability to evaluate therapeutics in the context of either personalized treatment or clinical trial format. Existing large libraries of PDXs, like the proprietary collection of >3000 PDXs^14,15,16,17, are therefore suitable for the rapid generation of libraries of tumor organoids (PDX-derived organoids, or PDXO), resulting in a matched library of paired PDX and PDXO models. This report describes the procedure to create and characterize colorectal cancer PDXO-CR2110 in relation to its parental PDX-CR2110 model¹⁶.

Protocol

All the protocols and amendment(s) or procedures involving the care and use of animals were reviewed and approved by the Crown Bioscience Institutional Animal Care and Use Committee (IACUC) prior to conducting the studies. The care and use of animals was conducted in accordance with AAALAC (Association for Assessment and Accreditation of Laboratory Animal Care) International guidelines as reported in the Guide for the Care and Use of Laboratory Animals, National Research Council (2011). All animal experimental procedures were under sterile conditions at SPF (specific pathogen-free) facilities and conducted in strict accordance with the Guide for the Care and Use of Laboratory Animals from different government institutions (e.g., The National Institutes of Health). The protocols were approved by the Committee on the Ethics of Animal Experiments at the facility institution (e.g., institutional IACUC Committee).

1. Preparation for tumor transplantation

1. Animal housing
   1. House Balb/c nude mice (n=5) in individual ventilated cages, at 20-26 °C, 30-70% humidity, and a lighting cycle of 12-h light/12-h dark, with corn cob bedding changed weekly, and irradiation sterilized dry granule food plus sterile drinking water ad libitum.
2. Donor tumor fragment preparation
   1. Closely monitor tumor-bearing donor mice for body weight (BW, via weighing balance), and tumor volume (TV, by caliper measurement).
   2. When TV reaches 800-1000 mm³, euthanize the tumor-bearing animals in a biohazard hood.
      1. Place mice in a euthanasia chamber with a lid that delivers CO₂ gas into the chamber. Discharge gas into the chamber at a flow rate that produces rapid unconsciousness with minimal distress to the animal. The optimum flow rate for CO₂ is around 2-2.5 Lpm.
      2. Ensure euthanasia by observing that the animals do not regain consciousness.
      3. After apparent clinical death, maintain gas flow for >1 min to minimize the possibility that an animal may recover.
   3. Sterilize the skin around the tumor using iodophor swabs. Collect tumors by removing adjacent non-tumor tissues and placing in a Petri dish containing 20 mL of PBS, pre-chilled (4 °C) prior to euthanasia.
   4. Wash the tumors with PBS in another Petri dish to remove blood components followed by cutting in half and removing any extra skin, blood vessels, calcification and/or necrosis.
   5. Place only intact tumor pieces into a sterile 50 mL centrifuge tube with 20 mL of PBS, prior to transporting to a separate animal room for transplantation.

2. Subcutaneous tumor growth

1. Subcutaneous inoculation of tumor piece into immunocompromised mice
   1. Cut the PDX tumor into 2 mm pieces with a scalpel, and place each into trocars for subcutaneous (SC) implantation.
   2. Anesthetize the recipient animals with 5% isoflurane (maintained by a nose cone at 1%). The animals relax, losing their righting reflex and eventually becoming immobile and unresponsive to pain. Fix the anesthetized mice onto an experiment board in the right lateral position and sterilize with iodophor swabs, particularly the areas surrounding the site of tumor inoculation.
   3. On left flank skin just cranial to the hip, make a 0.5 cm incision with a scalpel and create a tunnel under the skin towards the forelimb, 2-3 cm, using blunt forceps.
   4. Aseptically transfer one cube of tumor fragment per inoculation site from the medium and place deep inside the subcutaneous tunnel. Visually confirm position of the fragment prior to closure of wound with wound clips.
   5. Monitor the tumor implanted mice (5) until they become conscious to maintain sternal recumbence, and then return them to their cage only after their full recovery from anesthesia.
2. Tumor-bearing mice health monitoring
   1. Check water and food consumption daily and record body weight weekly.
   2. Check the mice during routine monitoring. Record any effects on mobility, breathing, grooming and general appearance, food and water consumption, BW gain/loss, ascites, etc.
   3. Measure TV twice weekly using calipers and express in mm³ per: TV = 0.5 a × b², where a and b are the length and width of the tumor, respectively.
   4. Sacrifice animals to collect samples when any of the following signs appear: BW loss >20%; impaired mobility (not able to eat or drink); unable to move normally due to significant ascites or enlarged abdomen; effort in respiration; death.

3. Necropsy and tumor harvest

1. When tumor volume reaches 200-800 mm³, euthanize mice per approved protocols (see step 1.2.2).
2. Collect tumor tissues by removing adjacent non-tumor tissues, followed by placing the tissue in a 50 mL plastic tube with AD+++ (on ice) before dissociation.

4. Preparation for PDX-derived organoid culture

NOTE: All the following steps were performed inside a biosafety cabinet per tissue culture standard guidelines. Keep pre-warmed stocks of 96-, 24-, and 6-well plates in a 37 °C incubator before use.

1. Reagent preparations
   1. Prepare basement membrane extract (BME) solution (growth factor reduced, Phenol Red-free). Keep 10 mL of BME in a 4 °C refrigerator overnight. Once thawed, swirl the BME bottle to ensure dispersion.
   2. Prepare base media/washing buffer AD+++. Add 5 mL of 200 mM L-glutamine, 1 M HEPES and Pen/Strep to Advanced DMEM/F12 media by pipetting with a 5 mL pipette.
   3. Prepare colon organoid medium as described by Sato et al.¹⁸ through supplementing base media with N-Ac (1 mM), A83-01 (500 nM), B27 (1x), EGF (50 ng/mL), Noggin (100 ng/mL), Nicotinamide (10 mM), SB202190 (10 nM), R-spondin (500 ng/mL), L-glutamine (2 mM), HEPES (10 µM), penicillin-streptomycin (1x) and Y-27623 (10 µM)¹⁹.
   4. Prepare AD+++Digestion medium: 10 mL of 1x organoid culture media with 500 µL of collagenase type II (20 mg/mL) and 10 µL of RhoKI Y-27632 (10 mM).
2. Tumor Dissociation²⁰
   1. Transfer the tumor in a 50 mL plastic tube to a 10 cm Petri dish. Take a macroscopic photograph alongside a ruler and record a description of its conditions (i.e., size, fat tissues, vascularisation, necrosis, etc.).
   2. Remove excess AD+++ by aspiration, and cut the tumor tissue into small pieces by scissors followed by transferral of 1-2 pieces into a 2 mL microtube for snap freezing on dry ice. Store at -80 °C for genomic profiling. Mince the remaining pieces into finer pieces by scissors before transferral to a 50 mL plastic tube using AD+++.
   3. Wash minced tissue 2-3 times by 35 mL of AD+++, followed by addition of 10 mL of digestion medium (see step 4.1.4) and placement on an orbital shaker at 4 x g for 1 h at 37 °C.
   4. Homogenize the digested tissue by pipetting up and down using a 5 mL sterile plastic pipette, followed by addition of 20 mL of AD+++ and filtration by 100 µm cell strainer.
   5. Wash the pass-through twice with AD+++ (spin at 450 x g for 5 min), followed by resuspension in BME (add 4x volume of BME to the pellet for suspension) and keep on ice¹⁹.
3. Preparation of organoid culture
   1. Add the BME cell suspension into 6-well plate in multiple drops to a total of 200 µL per well.
   2. Transfer the plate to a 37 °C incubator. After 30 min, the gel drops solidify.
   3. Add 2 mL of organoid media to each well, with the representative drops recorded by microscopic photography before transferring to an incubator (37 °C and 5% CO₂).
   4. Maintain the organoid cultures with medium change every 3-4 days, and passage at a 1:2 ratio every 7 days or depending on their growth and density.

5. Histopathology and next generation sequencing (NGS) analysis

1. Histopathology
   1. Collect organoids from the well with the existing medium using a P1000 pipette, followed by centrifugation (spin at 450 x g for 5 min), washing with PBS and fixation in 10% formalin for 1 h.
   2. Place the fixed organoids in 100% gelatin at the bottom of 50 mL conical tube, followed by routine tissue processing and embedding.
   3. Perform haematoxylin–eosin (H&E) staining using standard protocols on 4 mm paraffin sections.
2. RNAseq and whole exome sequencing
   1. Collect organoids from the well with the existing culture medium using a P1000 pipette, followed by centrifugation using a microcentrifuge at maximum speed (12,000 x g) for 5 min at 4 °C.
   2. Collect the pellet by removing the medium supernatant to ensure no visible BME was present, followed by snap freezing in a microtube (dry ice) and then transfer to a -80 °C freezer.
   3. Extract RNA or DNA using standard procedure from manufacturers and perform NGS analysis for both RNAseq and whole exome sequencing (WES).

6. IC₅₀ assay²⁰

1. Organoid seeding in 384-well plate for IC₅₀ assay
   1. Dissociate organoids in BME drops from each well (digesting BME) by adding 20 µL of 100x dispase solution to each well (6-well plate), which contained 2 mL of organoid medium, followed by 30 min of incubation at 37 °C.
   2. Pipette digested organoids from all wells through a 70 µm filter into a 50 mL plastic tube to collect the organoids.
   3. Count the organoids under microscopy for the determination of organoid concentration. Suspend the organoids using culture medium, before adding BME to reach final concentration of 5% (v/v) on ice.
   4. Add 50 µL of the organoid suspension into each 384-well plate with the liquid dispenser, according to the plate map with a seeding density of 200 CR2110 PDXOs per well in corresponding organoid culture medium.
2. Cisplatin and irinotecan treatment
   1. Use cisplatin (with the highest concentration of 100 µM) and “irinotecan” (with the highest concentration of 10 µM). Add SN-38 (a metabolite of irinotecan, as opposed to irinotecan which is usually used for in vivo studies) to each well according to the drug dilution scheme for 9 doses, in serial dilution by digital dispener.
   2. Create the platemap using the digital dispenser software tool. Include a negative control vehicle with 100% viability and postive control of 5 µM staurosporine, which showed 0% viability.
   3. Place the drug-treated 384-well plates back into 37 °C incubator.
3. Determination of organoid cell viability after drug treatment
   1. At the end of the 5 days of drug treatment, determine organoid cell viability using luminescent cell viability reagents as per the manufacturer’s recommended procedure. Add luminescent reagent into each well with the liquid dispener and mix for 5 min on a plate shaker, followed by a 30 min incubation at room temperature in dark.
   2. Record the luminescent signal on a luminescence multi-well plate reader.
   3. Calculate the normalized viabilities of each well using the raw readings from the plate reader and create a dose-response curve and IC₅₀ values by nonlinear curve fitting.

Results

Morphology of PDXOs, typical of organoids under light microcopy, and consistent with parental PDX per H&E staining
Under light microscopy, PDXO-CR2110 demonstrates typical cystic morphology (Figure 1A), as described previously for patient-derived organoids (PDO), evidence supporting the similarity between PDXO and PDO under the same culture conditions.

Histopathological examination by H&E staining reveals that the tissue structures and...

Discussion

The preliminary data for PDX-/PDXO-CR2110 in this report supports the biological equivalence between PDX and its derivative, PDXO, with regards to genomics, histopathology and pharmacology, since both models represent the disease forms from the original CSC of patient. Both models are patient-derived disease models, potentially predictive of the clinical response of patients^10,11,12,21. The mat...

Materials

List of materials used in this article

Name	Company	Catalog Number	Comments
Advanced DMEM/F12	Life Technologies	12634028	Base medium
DMEM	Hyclone	SH30243.01	Washing medium
Collagenese type II	Invitrogen	17101015	Digest tumor
Matrigel	Corning	356231	Organoid culture matrix (Basement Membrane Extract, growth factor reduced)
N-Ac	Sigma	A9165	Organoid culture medium
A83-01	Tocris	2939	Organoid culture medium
B27	Life Technologies	17504044	Organoid culture medium
EGF	Peprotech	AF-100-15	Organoid culture medium
Noggin	Peprotech	120-10C	Organoid culture medium
Nicotinamide	Sigma	N0636	Organoid culture medium
SB202190	Sigma	S7076	Organoid culture medium
Gastrin	Sigma	G9145	Organoid culture medium
Rspondin	Peprotech	120-38-1000	Organoid culture medium
L-glutamine	Life Technologies	35050038	Organoid culture medium
Hepes	Life Technologies	15630056	Organoid culture medium
penicillin-streptomycin	Life Technologies	15140122	Organoid culture medium
Y-27632	Abmole	M1817	Organoid culture medium
Dispase	Life Technologies	17105041	Screening assay
CellTiter-Glo 3D	Promega	G9683	Screening assay (luminescent ATP indicator)
Multidrop dispenser	Thermo Fisher	Multidrop combi	Plating organoids/CellTiter-Glo 3D addition
Digital dispener	Tecan	D300e	Compound addition
Envision Plate reader	Perkin Elmer	2104	Luminescence reading
Balb/c nude mice	Beijing HFK Bio-Technology Co
RNAeasy Mini kit	Qiagen	74104	tRNA purification kit
DNAeasy Blood & Tissue Kit	Qiagen	69506	DNA purification kit
Histogel	Thermo Fisher	HG-4000-012	Organoid embedding