CEA expression heterogeneity and plasticity confer resistance to the CEA-targeting bispecific immunotherapy antibody cibisatamab (CEA-TCB) in patient-derived colorectal cancer organoids
The T cell bispecific antibody cibisatamab (CEA-TCB) binds Carcino-Embryonic Antigen (CEA) on cancer cells and CD3 on T cells, which triggers T cell killing of cancer cell lines expressing moderate to high levels of CEA at the cell surface. Patient derived colorectal cancer organoids (PDOs) may more accurately represent patient tumors than established cell lines which potentially enables more detailed insights into mechanisms of cibisatamab resistance and sensitivity.
We established PDOs from multidrug-resistant metastatic CRCs. CEA expression of PDOs was determined by FACS and sensitivity to cibisatamab immunotherapy was assessed by co-culture of PDOs and allogeneic CD8 T cells.
PDOs could be categorized into 3 groups based on CEA cell-surface expression: CEAhi (n = 3), CEAlo (n = 1) and CEAmixed PDOs (n = 4), that stably maintained populations of CEAhi and CEAlo cells, which has not previously been described in CRC cell lines. CEAhi PDOs were sensitive whereas CEAlo PDOs showed resistance to cibisatamab. PDOs with mixed expression showed low sensitivity to cibisatamab, suggesting that CEAlo cells maintain cancer cell growth. Culture of FACS-sorted CEAhi and CEAlo cells from PDOs with mixed CEA expression demonstrated high plasticity of CEA expression, contributing to resistance acquisition through CEA antigen loss. RNA-sequencing revealed increased WNT/β-catenin pathway activity in CEAlo cells. Cell surface CEA expression was up-regulated by inhibitors of the WNT/β-catenin pathway.
Based on these preclinical findings, heterogeneity and plasticity of CEA expression appear to confer low cibisatamab sensitivity in PDOs, supporting further clinical evaluation of their predictive effect in CRC. Pharmacological inhibition of the WNT/β-catenin pathway may be a rational combination to sensitize CRCs to cibisatamab. Our novel PDO and T cell co-culture immunotherapy models enable pre-clinical discovery of candidate biomarkers and combination therapies that may inform and accelerate the development of immuno-oncology agents in the clinic.
KeywordsCibisatamab CEA Immunotherapy Patient-derived organoids WNT/β-catenin
Chimeric Antigen Receptor
Carcino Embryonic Antigen
Carcino Embryonic Antigen-T Cell Bispecific
Effector to Target
enhance Green Fluorescent Protein
Fluorescence-Activated Cell Scanning
Gene Set Enrichment Analysis
Mean Fluorescence Intensity
Peripheral Blood Mononuclear Cells
Programmed Death Ligand 1
Patient Derived Organoid
T Cell Receptor
Colorectal cancer (CRC) is the third most common cause of cancer related mortality worldwide . Median overall survival for patients with metastatic CRC has increased to over 24 months since the introduction of anti-vascular endothelial growth factor (VEGF) and anti-epidermal growth factor (EGFR) targeted therapies . Trifluridine-tipiracil (TAS102) and the multi-kinase inhibitor regorafenib are recently developed third line therapy options but their survival benefit is only modest [3, 4]. Thus, new therapies are needed to further improve outcomes of patients with metastatic CRC.
Checkpoint-inhibiting immunotherapies recently led to substantial increase in survival in some tumor types. These include hypermutated microsatellite instable (MSI) CRCs [5, 6] but checkpoint inhibitors showed no activity in microsatellite stable (MSS) CRCs. High numbers of mutation encoded neo-antigens in MSI CRCs are thought to foster spontaneous immune response with increased cytotoxic CD8 T cell infiltrates that are kept in check by cancer cells through upregulation of PD-L1 . Unfortunately, only ~ 5% of metastatic CRCs display the MSI phenotype . Thus, benefit from checkpoint inhibitors is currently restricted to a small subgroup of CRC patients .
The T cell bispecific antibody cibisatamab (CEA-TCB) is a novel immunotherapy that redirects T cells independently of their T cell receptor specificity to tumor cells expressing the carcinoembryonic antigen (CEA) glycoprotein at the cell surface . A major advantage of T cell redirecting bispecific antibodies is that they mediate cancer cell recognition by T cells independently of neoantigen load. CEA is overexpressed on the cell surface of many colorectal cancers and cibisatamab is hence a promising immunotherapy agent for non hypermutated MSS CRCs.
Cibisatamab has a single binding site for the CD3 epsilon chain on T cells and two CEA binding sites which tune the binding avidity to cancer cells with moderate to high CEA cell surface expression . This avoids targeting of healthy epithelial cells with low CEA expression levels, which are physiologically present in some tissues. Binding of cibisatamab to CEA on the surface of cancer cells and of CD3 on T cells triggers T cell activation, cytokine secretion and cytotoxic granule release. The phase I trial of cibisatamab in patients with CEA expressing metastatic CRCs that had failed at least two prior chemotherapy regimens showed antitumor activity with radiological shrinkage in 11% (4/36) and 50% (5/10) of patients treated with monotherapy or in combination with PD-L1-inhibiting antibodies, respectively [12, 13]. Based on these results, CEA is one of the most promising target antigens for immunotherapy in MSS CRCs. Although some patients in this dose escalation trial were treated with a dose below the final recommended dose, the response rates nevertheless indicate that a subgroup of tumors is resistant to treatment.
Molecular mechanisms of cibisatamab activity have been investigated in CRC cell lines in vitro using killing assays with peripheral blood mononuclear cells . This identified CEA expression as a major determinant of cibisatamab sensitivity as only cell lines expressing moderate to high CEA levels were susceptible to T cell mediated killing. In contrast, cibisatamab sensitivity was independent of the presence of mutations in CRC driver genes such as APC, TP53, KRAS and BRAF.
Recently developed protocols allow the expansion and long term propagation of cancer cells as so called patient derived organoids (PDOs) from CRC biopsies . PDOs have been suggested to better represent the biological characteristics of patient tumors than cancer cell lines which were often established decades ago and have undergone changes during long term culture on plastic. The ability to rapidly generate model systems from patients furthermore enables matching of disease stage and prior treatment history to those of patients in whom novel drugs are clinically tested.
Identification of resistance mechanisms for novel immunotherapies in patient-relevant preclinical models should define candidate biomarkers for the identification of sensitive patient subgroups or of combination therapy strategies that enhance efficacy by co-targeting of resistance pathways. This could maximize trial success rate and prevent drug attrition, which remains common for new cancer drugs in the absence of biomarkers. The aim of this study was to investigate mechanisms of resistance to cibisatamab immunotherapy beyond those identified in cell lines by using PDO models from treatment refractory metastatic CRCs. To this end, we established seven PDOs from chemotherapy resistant metastatic CRCs and one from a treatment naïve primary CRC and developed an in vitro co-culture assay with CD8 T cells to assess cibisatamab efficacy.
Material and methods
Human samples and cell lines
Imaging-guided core biopsies from metastatic colorectal cancers that had been treated with at least two prior lines of chemotherapy were obtained from the Prospect C and Prospect R trials (Chief investigator: D. Cunningham, UK national ethics committee approval numbers: 12/LO/0914 and 14/LO/1812, respectively). One endoscopic biopsy from a treatment naïve primary colorectal cancer was obtained from the FOrMAT trial (Chief investigator: N. Starling, UK national ethics committee approval number 13/LO/1274). Trials were run at the Royal Marsden Hospital and all patients provided written informed consent before trial inclusion. Anonymized buffy coats from healthy donors were obtained from the local blood bank (National ethics committee approval number 06/Q1206/106) or through the Improving Outcomes in Cancer biobanking protocol at the Barts Cancer Institute (Chief investigator: T. Powles, UK national ethics committee approval number: 13/EM/0327) from individuals providing written informed consent. DLD-1 and MKN-45 cell lines were obtained from the American Type Culture Collection and were maintained in RPMI 1640 medium supplemented with 10% FBS, 1X Glutamax and 100units/ml penicillin/streptomicin (Thermo Fisher).
Generation of patient derived organoids
PDO cultures from CRC-01, CRC-02 and CRC-06 were established directly from core biopsies by rough chopping followed by embedding in growth factor reduced Matrigel (Corning). Very small biopsy fragments were available from CRC-03, CRC-04, CRC-05, CRC-07 and CRC-08 and these were first grafted subcutaneously or under the kidney capsule of female CD1 nude mice by the Tumour Profiling Unit at the Institute of Cancer Research (Home office licence number PD498FF8D). Mice were culled once tumors had grown and tumors were removed and dissociated in a gentleMAX Octo dissociator using the Human Tumour Dissociation Kit (Miltenyi Biotec). Mouse cells were magnetically removed using the Mouse Cell Depletion Kit (Miltenyi Biotec), and purified human tumour cells were embedded into growth factor reduced Matrigel. PDOs were expanded in Matrigel as described  using Advanced DMEM/F12 media supplemented with 1X Glutamax, 100 units/ml penicillin/streptomycin, 1X B27, 1X N2, 10mM HEPES (all Thermo Fisher), 1mM N-acetyl cysteine, 10mM nicotinamide, 10uM SB202190, 10nM gastrin, 10uM Y27632 (Sigma Aldrich), 10nM prostaglandin E2, 500nM A-83-01, 100ng/ml Wnt3a (Biotechne), 50ng/ml EGF (Merck), 1μg/ml R-Spondin, 100ng/ml Noggin, and 100ng/ml FGF10 (Peprotech). After at least 2 months of continuous growth in the matrigel matrix (minimum of 12 passages), the PDOs were first eGFP tagged (see below) and then adapted to grow in DMEM/F12 (Sigma Aldrich) with 20% fetal bovine serum (FBS), 1X Glutamax, 100 units/ml penicillin/streptomycin containing 2% Matrigel. PDO cultures were maintained in these conditions and used as required for T cell co-culture assays and FACS analysis. Genetic analyses of colon cancer driver genes were performed on each PDO line and these were identical to the mutations that had been identified in the matched tumor biopsies.
Labelling of PDOs with nuclear eGFP
The nuclei of PDOs were labelled by introducing an eGFP tagged histone 2B construct (pLKO.1-LV-H2B-GFP)  to enable cell quantification by automated microscopy. For virus generation, HEK-293T cells were cultured in DMEM supplemented with 10%FBS, 1XGlutamax and 100units/ml penicillin/streptomycin. Lentiviral particles were produced by overnight transfection with a plasmid mixture containing 9 μg of pLKO.1-LV-H2B-GFP, 2.25 μg of psPAX2 packaging plasmid (gift from Didier Trono; Addgene plasmid #12260; http://n2t.net/addgene:12260; RRID:Addgene_12,260) and 0.75 μg of pMD2.G envelope plasmid (gift from Didier Trono; Addgene plasmid # 12259; http://n2t.net/addgene:12259; RRID:Addgene_12,259) using TransIT-293 transfection reagent (Mirus). The cells were media changed the following day, virus harvested after 24 h and passed through a 0.45uM filter before use. For lentiviral transduction PDOs were harvested from the cultures in Matrigel and dissociated to single cells using TrypLE Express (Thermo Fisher), and pelleted. The pellets were resuspended in media with the addition of virus and 1nM polybrene (Sigma Aldrich) and centrifuged at 300g for 1 h. The samples were resuspended and plated in culture for between 6 h and overnight, before replacing the media. Following recovery and expansion, eGFP positive cells were sorted by flow cytometry and further expanded before use.
Surface CEA expression analysis by flow cytometry
Cell lines were harvested using enzyme-free Cell Dissociation Buffer (Thermo Fisher) and PDOs with TrypLE Express (Gibco). 2 × 105 cells were stained with 20nM of the human anti-human CEA antibody CH1A1A (Roche) and 25μg/ml of the R-Phycoerythrin conjugated secondary antibody AffiniPure F(ab’)2 Fragment Goat Anti-Human IgG, Fcγ Fragment Specific (Stratech). DRAQ7 (Biostatus) staining was included for dead cell exclusion. CEA expression was analysed on a Sony SH800 flow cytometer. Gate boundaries were set at the trough between high and low CEA populations in PDOs with mixed CEA expression and identical gates were used across all samples. The percentage of CEAhi and CEAlo populations and mean fluorescence intensities (MFI) were calculated for each PDO.
CEA expression analysis in human protein atlas samples
Microscopic images of 11 CRC samples stained by the Human Protein Atlas (www.proteinatlas.org) with the rabbit polyclonal antibody HPA019758 (Sigma Aldrich) which has been validated against RNA expression data, immunofluorescence staining with an independent antibody and by Western blot were downloaded and assessed for expression heterogeneity by two pathologists (K. von Loga and B. Challoner).
CD8 T cells expansion from peripheral blood mononuclear cells
Peripheral Blood Mononuclear Cells (PBMCs) were isolated from buffy coats with Ficoll-Paque according to the manufacturer’s protocol (GE Healthcare). CD8 T cells were isolated from PBMCs with Human CD8 Dynabeads FlowComp (Thermo Fisher). The purity of CD8 T cells was assessed by flow cytometry (Alexa Fluor 488 anti-human CD8, Sony Biotechnology) and only populations with at least 90% CD8 positive cells were used for expansion with the CD3/CD28 Dynabeads Human T-Activator kit (Thermo Fisher) in RPMI 1640 supplemented with 10% FBS (Biosera), 1X Glutamax, 100units penicillin/streptomycin and 30 U/mL IL-2 (Sigma Aldrich) following the manufacturer’s protocol.
Co-culture of PDOs and CD8 T cells
PDOs were harvested with TrypLE Express and neutralised with DMEM/F12 Ham medium (Sigma Aldrich) with 10% FBS. Cells were filtered through a 70um filter, counted and re-suspended in phenol-red free RPMI medium (Thermo Fisher) supplemented with 10% FBS (Biosera), 1XGlutamax and 100units penicillin-streptomycin. On day 0, 5000 tumor cells per well of a 96 well-plate (Corning Special Optics Microplate) were plated. CD8 T cells were added on day 1 at the indicated effector to target (E:T) ratios with 20nM of cibisatamab or 20nM of the untargeted negative control antibody DP47-TCB (both provided by Roche). Tumor cells without CD8 T cells and without antibody were also included as controls. All conditions were plated in triplicates and at least 3 different healthy donors were tested on each of the 8 PDOs.
Cancer cell growth assessment by immunofluorescence microscopy
The GFP confluence was quantified every 48h–72h over a 10-day period using the GFP confluence application on the Celigo Imaging Cytometer (Nexcelom Bioscience). GFP confluence analysis was able to track the growth of GFP positive PDO cells over multiple timepoints without erroneously counting the T cells in the co-culture. Confluence analysis was furthermore superior to the counting of cell nuclei which generated inaccurate results in areas of high cancer cell density such as the PDO centre. The main advantage of confluence analysis over measuring spheroid diameters is the ability to track even the the growth of PDOs showing highly variable shapes. Growth curves were generated with CD8 T cells from three different healthy blood donors. The percentage growth reduction was calculated from readings taken between days 7 to 9, before PDOs showed growth retardation, likely due to exhaustion of the growth media. In order to calculate the percentage of growth reduction, confluence at day 1 was subtracted and the confluence in wells treated with the DP47-TCB control antibody at the endpoint was set to 100%.
Flow sorting of CEAhi and CEAlo cells
PDOs cells were harvested with TrypLE Express, filtered through a 70um filter to obtain a single cell solution and 2 × 106 cells were stained with DAPI for dead cell exclusion, 20nM of the CH1A1A antibody (Roche) and 25μg/ml of the R-Phycoerythrin conjugated secondary antibody (Stratech) and sorted in CEAhi and CEAlo cells in an ARIAIII cytometer (BD Biosciences) in the FACS core facility at the Institute of Cancer Research. Cells were collected in cold DMEM supplemented with 10% FBS and pellets were frozen at -80°C after centrifugation for RNA-sequencing. CEAhi and CEAlo cells sorted from CRC-06 and CRC-08 were also grown for 1 month in DMEM/F12 Ham medium with 20% FBS, penicillin/streptomycin and 2% Matrigel.
Gene expression analysis
Total RNA was extracted from frozen pellets of flow sorted of CEAhi and CEAlo populations from CRC-03, CRC-06 and CRC-08 using RNAeasy Plus (Qiagen) and quantified with Qubit RNA High Sensitivity assay (Thermo Fisher). RNA sequencing libraries were prepared using the QuantSeq 3′-mRNA-Seq Library Prep Kit FWD for Illumina (Lexogen) using the manufacturer’s protocol. A minimum of 5 ng input RNA was used from each sample and qPCR was performed on all samples before PCR amplification of the library to determine optimal cycle number following the manufacturer’s recommendations. Final libraries were quantified in duplicate using Qubit-HS and Bioanalyzer High Sensitivity (Agilent) before pooling. Libraries were sequenced with 100 single read cycles on an Illumina HiSeq2500 in rapid mode. Alignment and gene counting were performed on the Lexogen QuantSeq data analysis pipeline on the Bluebee cloud. Annotation data on the GRCh38.p12 genome assembly was exported from Ensembl with Biomart. The ID’s of protein coding genes were identified using the gtf file filtered on the ‘gene_biotype’ field. The Quantseq raw count data were then filtered for this gene set and the Ensembl ID’s converted to gene symbol using the Homo.sapiens Bioconductor package. Lowly expressed genes containing fewer than 10 counts were removed from the dataset. The count data were then normalised using the estimateSizeFactors and counts functions from the DESeq2 Bioconductor package .
WNT/β-catenin pathway inhibition assay
105 PDO cells/well were seeded in 12 well plates and allowed to attach overnight. Media were changed and cells were treated with DMSO control or with 10uM tankyrase inhibitor (Compound 21, kindly provided by Prof Lord)  or 10uM porcupine inhibitor (LGK-974, SelleckChem) for 3 days. Cells were harvested using TrypLE Express, stained for CEA with the CH1A1A primary antibody and the R-Phycoerythrin conjugated secondary antibody and analyzed by FACS as described above.
Pearson correlation analysis and the paired t-tests were performed with the GraphPad Prism software. All p values are two tailed. Gene set enrichment analysis was performed with the GSEA software V3.0 using 5000 gene set permutations and the Hallmarks V6.2 gene set collection .
Generation of patient derived organoids from colorectal cancers
CRC PDOs were established as 3D cultures in Matrigel a) directly from core biopsies from three chemotherapy resistant metastatic CRCs (CRC-01, CRC-02, CRC-06), b) from small core biopsies of four chemotherapy resistant metastatic CRCs which were first expanded as xenografts in immunodeficient mice (CRC-03, CRC-04, CRC-05, CRC-07) and c) from an endoscopic biopsy taken from a treatment naive primary CRC (CRC-08). Each PDO was continuously grown for at least 2 months in Matrigel to test for long term viability. They were labelled with a lentivirus encoding a histone tagged nuclear enhanced green fluorescent protein (eGFP) and were subsequently transferred into culture conditions with 2% Matrigel dissolved in growth medium. Matrigel does not form a solid culture matrix at this dilution and allows PDOs to attach to the bottom of the plastic plate. These culture conditions facilitate interaction with T cells and allow monitoring of PDO growth with wide field fluorescence light microscopy.
CEA expression heterogeneity in patient derived CRC organoids
The most striking CEA expression heterogeneity was detected in 4 PDOs (CRC-02, CRC-03, CRC-04 and CRC-08) which each contained large subpopulations of CEAhi and CEAlo cells. The MFI of the CEAhi subpopulations were similar to MKN-45 in two PDOs (CRC-03, CRC-04) and moderately lower in two others (CRC-02, CRC-08). A proportion of the CEAlo cells in each of these four PDOs showed CEA expression levels which were as low as in the DLD-1 cell line, demonstrating heterogeneity across a broad range of CEA expression levels.
The heterogeneous CEA expression profiles of these PDOs is reminiscent of the CEA expression heterogeneity which has been described in CRC samples from patients . We furthermore evaluated CRC tissue samples that had been stained with a validated CEA antibody by the Human Protein Atlas  and this also revealed CEA expression heterogeneity in 6/11 samples (54%; Fig. 1c). Importantly, similar expression heterogeneity to that observed in PDO samples was not present within DLD1 or MKN-45 cells and bimodal expression profiles have, to our knowledge, not previously been described in CRC cell lines. This supports the notion that PDOs better represent the molecular heterogeneity of colorectal cancers than established cell lines.
Cibisatamab sensitivity of PDOs in an allogeneic T cell co-culture assay
We next tested the four PDOs with mixed CEA expression. Each of these continued to proliferate despite treatment with cibisatamab and T cells, with only a moderate reduction of the cancer cell growth rate compared to controls (Fig. 3a and b). Thus, PDOs with mixed CEA expression only showed a partial response to this CEA targeting immunotherapy. Correlation analysis of the achieved growth reduction with the fraction of CEAhi cancer cells in each PDO showed a strong and significant correlation (r = 0.9152, 95% CI: 0.593 to 0.9848; p = 0.0014; Fig. 3c). This substantiates that only the CEAhi population is sensitive whereas CEAlo cells continue to grow and promote resistance.
Taken together, CEA expression was frequently heterogeneous, showing a bimodal pattern in 50% of PDOs which has not been observed in cancer cell lines, and this phenomenon was associated with poor susceptibility to cibisatamab treatment.
CEA expression plasticity in CRC PDOs
The sorted CEAlo cells had each re-established CEAhi subpopulations which were between 47.9 and 54.1% of the size of the CEAhi population in the parental PDOs (Fig. 4a). Sorted CEAhi cells also re-established CEAlo cell populations but with noticeable different conversion rates in the two PDOs. CEAhi cells from CRC-08 had re-generated 58.1% of the CEAlo population size present in the parental cells whereas those from PDO CRC-06, which harbored a much larger proportion of CEAlo cells in the parental population than CRC-08, had re-generated a CEAlo population that was 98.6% of the size of the parental CEAlo population. This demonstrates a high level of plasticity of CEA expression which rapidly re-establishes a heterogeneous population.
We next re-analysed the sensitivity to cibisatamab and CD8 T cell treatment in the cells that had been re-expanded from sorted CEAhi and CEAlo cells. Similar to the results obtained in parental PDOs with mixed CEA expression, treatment with cibisatamab had low efficacy (Fig. 4b), further corroborating that CEAlo cells confer resistance. This experiment shows that CEA expression is highly plastic in many PDOs which promotes population heterogeneity and cibisatamab resistance.
Identification of pathways regulating CEA expression
Our aim was to identify regulatory and potentially actionable pathways that control CEA expression and we hence focused subsequent analyses on the WNT/β-catenin signalling pathway. This pathway is genetically activated in the majority of CRCs, most frequently through mutations and loss of heterozygosity of the APC tumor suppressor gene and less commonly through mutations of other regulators of WNT signalling such as RNF43 or in β-catenin/CTNNB1 itself [21, 22]. Seven of the PDO samples harbored truncating mutations in the APC gene which result in gene products lacking six or seven of the seven β-catenin binding domains in the APC gene (Fig. 5d). Two independent APC mutations were identified in each of two PDOs (CRC-01, CRC-02). All three PDOs in which GSEA analysis had shown different WNT/β-catenin signatures activity in FACS sorted CEAhi and CEAlo subpopulations harbored APC mutations. This demonstrated that the WNT pathway remains regulated in these PDOs despite the presence of APC mutations, a phenomenon previously observed in CRC model systems and patient tumors [23, 24, 25]. Moreover, there was no association between the number of β-catenin binding domains that were inactivated by APC mutations and the fraction of CEAlo and CEAhi cells in these eight PDOs.
High WNT/β-catenin pathway activity and absence of CEA expression are features of the intestinal crypt bottom where intestinal stem cells reside  . ,Moreover, high WNT/β-catenin pathway activity is also a characteristic of colon cancer stem cells . However, the stem cell markers LGR5, CD133 or CD44 were not upregulated in CEAlo compared to CEAhi cells (Fig. 5e), suggesting that CEAlo cells do not represent a classical CRC stem cell population .
WNT/β-catenin pathway inhibition increases CEA expression
We finally investigated if pharmacological inhibition of the WNT/β-catenin pathway enhances CEA expression as predicted by these data. Three PDO lines with mixed CEA expression were treated with two different inhibitors of WNT signalling: a) the porcupine inhibitor LGK-974 which prevents WNT ligand secretion and hence autocrine and paracrine WNT-receptor activation and b) the tankyrase inhibitor compound 21 which inhibits the downstream WNT/β-catenin pathway by stabilizing the β-catenin destruction complex [17, 30]. Both compounds increased CEA expression and the CEAhi subpopulation in all three PDOs (Fig. 5f). The tankyrase inhibitor consistently led to a stronger increase of CEA expression than porcupine inhibitor treatment, perhaps suggesting a limited contribution of auto- or paracrine WNT ligands to pathway regulation in these cells. These results confirmed a role of WNT/β-catenin signalling as a regulator of CEA expression in CRC PDOs.
This analysis of cibisatamab immunotherapy in a co-culture model of allogeneic T cells and PDOs, established mainly from metastatic chemotherapy resistant CRCs, confirmed high cell surface CEA expression as a key determinant of treatment sensitivity in vitro. Importantly, in contrast to cell lines, we found that CEA expression is frequently heterogeneous within PDO populations, resulting in bimodal CEA expression patterns in its most extreme form. We furthermore demonstrated high phenotypic plasticity that enables CRC cells to switch between high and low CEA expression. These results are likely highly relevant for CEA targeting immunotherapies as all 4/8 PDOs with mixed CEA expression profiles were at least partially resistant to cibisatamab treatment in vitro.
The observation that FACS sorted CEAhi cells from the predominantly CEAlo PDO CRC-06 more rapidly converted back to the CEAlo state than those from the CEAmixed PDO CRC-08 furthermore suggest that differences in the transition rate from high to low CEA and vice versa may determine the abundance of CEAhi and CEAlo cells at the long term equilibrium. Moreover, gene expression profiles of CEAhi and CEAlo cells from individual PDOs demonstrated that cell surface expression of CEA is regulated at the gene expression level and negatively correlates with WNT/β-catenin pathway activity. CEA expression is tightly regulated in healthy colonic crypts where expression is absent at the crypt bottom that harbors intestinal stem cells and gradually increases in epithelial cells as they become more differentiated towards the top of the crypt. The activity of WNT/β-catenin signalling physiologically decreases along the same axis, from the highest levels at the crypt bottom to low signalling activity at the top of the crypt. Together with our results that demonstrate a negative correlation between CEA expression and a WNT/β-catenin activity signature in PDOs, this suggests that the regulation of CEA expression heterogeneity in PDOs and in healthy colon epithelial cells is similar.
We found no correlation between the degree of APC protein truncation by distinct mutations, which is likely to lead to different levels of β-catenin signalling pathway activation , with CEA expression levels or CEA heterogeneity. In addition, we showed that β-catenin signalling remains regulated in PDOs despite genetic activation through APC mutations. Preservation of WNT/β-catenin pathway regulation and heterogeneity despite genetic activation of the pathway have recently been shown in CRC cell lines and animal models and this has been attributed to a several cell intrinsic, autocrine and also stromal factors that influence multiple pathways converging on b-catenin [23, 24, 25]. Similar mechanisms may explain heterogeneity in these PDO models.
The upregulation of a signature of oxidative phosphorylation in CEAlo cells highlights further similarities to intestinal stem cells at the crypt bottom which are more dependent on oxidative phosphorylation than their more differentiated progeny towards the top of the crypt . Despite the gene expression similarities between CEOlo cells in PDOs and the crypt bottom where stem cells reside, specific genes which have frequently been associated with stemness in CRC were not upregulated in the CEOlo cells from our PDOs. This may indicate a dissociation of the mechanisms that regulate differentiation processes including CEA expression and stemness in PDOs from advanced and drug resistant tumours but this requires further investigation.
The critical role of CEA expression heterogeneity and plasticity as determinants of treatment resistance in our in vitro models may be relevant for the characterization of predictive biomarkers for CEA-targeting immunotherapies in CRC where heterogeneous CEA expression has been described. Moreover, finding strategies to increase CEA expression may increase the clinical responses of cibisatamab.
PDOs harboring predominantly CEAhi cells were highly sensitive to cibisatamab treatment in vitro but the low level of expression plasticity we observed may nevertheless enable gradual loss of the target antigen during prolonged treatment. The plasticity of CEA expression which re-establishes a CEAhi population after FACS sorting of CEAlo cells suggests that re-treatment with cibisatamab after a prolonged treatment break may lead to further responses. Phenotypic plasticity may furthermore be amenable to combination therapies which either increase CEA expression in the CEAlo population or which co-target vulnerabilities of the CEAlo subpopulations while also administering cibisatamab. Our results provided proof of principle that CEA expression can be pharmacologically perturbed and indicate WNT pathway inhibitors, which are in clinical development, as a potential strategy to boost CEA expression and increase therapeutic benefit from bispecific CEA-targeting antibodies. However, the WNT pathway has an essential role in the development and the homeostasis of many normal tissues in the human body. As a consequence, targeting of the WNT pathway has been challenging in preclinical models and clinical trials, particularly due to gastrointestinal toxicities . However, there is cautious optimism that a better understanding of WNT regulation in malignant cells and of the cross-talk between the WNT and other signaling pathways in cancer may enable the design of new molecules with a broader therapeutic window and lower toxicity . Our results also question whether CEAlo cells may be susceptible to inhibition of oxidative phosphorylation as an alternative strategy to address this subpopulation. Several CEA targeting immunotherapies beyond bispecific T cell redirecting antibodies are currently in preclinical or clinical development, including CEA vaccines and CEA targeting CAR T cells or TCR engineered T cells . CEA expression plasticity and heterogeneity are likely hindrances for each of these approaches. Together with the limited success that has so far achieved in MSS CRCs with checkpoint inhibiting immunotherapies alone, strategies to enhance CEA expression in combination with CEA targeting therapies appear promising to extend immunotherapy benefit to a larger proportion of CRC patients.
Finally, this study shows the potential of PDO and allogeneic T cell co-cultures as novel tools to dissect mechanisms of immunotherapy resistance in vitro. This addresses a major need in translational immunotherapy research, particularly as studies in immunocompetent animal models are often slow and expensive and sometimes even impossible as animal models are not available for all tumor types, or are incompatible with human-specific reagents, including many monoclonal antibodies. Allogeneic systems can be hampered by alloreactivity where donor T cells recognize MHC molecules on target cells as non-self. This can lead to high background killing activity that may impair assay sensitivity and specificity compared to autologous systems. Cancer cells alone as well as in co-culture with T cells but without antibody were included as controls in our assays. This allowed us to identify and exclude the small number of experiments in which alloreactivity impaired cancer cell growth. Using allogeneic T cells in PDO co-culture models hence represent a valid alternative strategy when autologous T cells are unavailable. These PDO T cell co-culture models can accelerate the discovery of immune-oncology candidate resistance mechanisms, biomarkers of efficacy and define rational combination therapy strategies for clinical testing. The ability of PDOs to represent intra-tumor heterogeneity to some degree, and the opportunity to establish them from tumors which match the stage and the treatment history of patients in which novel drugs are tested, are decisive advantages for pre-clinical discovery.
CEA expression heterogeneity is common in CRC PDOs from therapy resistant metastatic CRCs and this confers cibisatamab resistance in vitro. Whether CEA expression heterogeneity is associated with cibisatamab resistance should be investigated in clinical trial samples. CEA expression can be pharmacologically enhanced through WNT/β-catenin pathway inhibition, suggesting opportunities for combination therapies that should increase cibisatamab efficacy in the clinic.
We would like to thank all patients participating in the Prospect C, Prospect R and FOrMAT clinical trials, their families and the clinical research team at the Royal Marsden Hospital who supported the sample collection, Roche Glycart for providing reagents and Dr. Marina Bacac for insightful discussions.
The study was supported by charitable donations from Tim Morgan and by research funding from Cancer Research UK, a Wellcome Trust Strategic Grant (105104/Z/14/Z) to the Institute of Cancer Research Centre for Evolution and Cancer and by the Royal Marsden Hospital/Institute of Cancer Research NIHR Biomedical Research Centre for Cancer.
Availability of data and materials
Gene expression data of sorted CEAhi and CEAlo PDO subpopulations is provided in Additional file 1: Table S1. The bispecific antibodies cibisatamab (CEA-TCB) and DP47-TCB and the human anti human CEA antibody CH1A1A were provided by Roche Glycart under a material transfer agreement.
RGE, MS, BG, LJB and MG conceived the study and wrote the manuscript: RGE, MS, LJB, GS and BG performed experiments. BG, GS and AS established organoid cultures. RGE, MS, LJB, AW, KVL and MG analyzed the data. RP and FW provided support for FACS sorting and analysis. KK, JT, AB, CS, TP, DM, AM, SR, DW, IC, NS and DC provided human tissue or blood samples. NM and LJB performed RNA sequencing. LJB and AW processed the RNA sequencing data. All authors read and approved the final manuscript.
Ethics approval and consent to participate
Human samples were obtained from clinical trial and biobanking protocols which have been approved by the UK National Ethics Committee (Prospect C trial approval number: 12/LO/0914, Prospect R trial approval number: 14/LO/1812, FOrMAT trial approval number 13/LO/1274, Improving Outcomes in Cancer biobanking protocol approval number: 13/EM/0327, approval number for use of buffy coats from the blood bank: 06/Q1206/106). All individuals provided written informed consent for sample donation and use for research.
Consent for publication
All authors read the manuscript and consented to publication.
Dr. Gonzalez-Exposito was supported by a fellowship grant from the Spanish Society of Medical Oncology for Translational Research in Reference Centers that was funded by Roche (FSEOM/Roche). Dr. Gerlinger receives research funding from Merck KG.
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