Comparison of Human and Murine Enteroendocrine Cells by Transcriptomic and Peptidomic Profiling

Enteroendocrine cells (EECs) are specialized hormone-secreting cells in the intestinal epithelium that monitor the quality and quantity of ingested foods. They produce at least 20 different hormones, mostly peptides, that act in concert to coordinate digestion, peripheral nutrient disposal, and appetite through actions at local and distant target tissues. In the field of human metabolism, glucagon-like peptide 1 (GLP-1) and peptide YY (PYY) have raised particular interest because of their central and pancreatic actions controlling food intake and insulin secretion. GLP-1–based drugs are widely used for the treatment of type 2 diabetes and obesity, and new gut hormone–based therapeutics are under development, aiming to mimic the unrivalled effectiveness of gastric bypass surgery on weight loss and type 2 diabetes resolution (1).

Recent years have witnessed substantial progress in our understanding of murine EEC physiology, facilitated by the generation of transgenic mice with fluorescently labeled EECs that enable cell identification and functional characterization through a range of approaches including fluorescence-activated cell sorting (FACS), transcriptomics, and live-cell imaging (2–7). Our knowledge of human EECs, however, is limited by a lack of methods to identify and characterize this scattered cell population that only comprises ∼1% of the intestinal epithelium (2). A number of G-protein–coupled receptors (GPCRs) have been identified and characterized in murine EECs that represent promising candidates for therapeutic approaches to enhance endogenous gut hormone secretion, but tools to predict the translatability of these findings from mouse to humans would be a major advance in this field (8).

The objectives of this study were to generate transcriptomic profiles of human EECs and to compare mouse and human EECs at the transcriptomic and peptidomic levels. We sequenced EECs from humans and mice at a depth sufficient for the identification of low-abundance transcripts, including GPCRs and ion channels. With liquid chromatography–tandem mass spectrometry (LC-MS/MS), we mapped the exact sequences of different gut peptides produced along the gastrointestinal (GI) tract in humans and mice.

This study was conducted in accordance with the principles of the Declaration of Helsinki and good clinical practice. Human ethics approvals were given by Cambridge Central and South Research Ethics Committees (ref: 09/H0308/24, 16/EE/0338, 15/EE/0152) and the INSERM ethics committee and Agence de la Biomédecine (ref: PFS16–004). Animal work was regulated under the Animals (Scientific Procedures) Act 1986 Amendment Regulations 2012 and conducted following ethics review by the University of Cambridge Animal Welfare and Ethical Review Body.

Jejunal tissue was obtained from 11 human participants (Supplementary Table 1). Samples of human jejunum discarded during surgery were collected during total gastrectomy for treatment or prophylaxis of gastric cancer or Roux-en-Y gastric bypass for obesity. All were from the point of enteroenterostomy 50 cm distal to the ligament of Treitz. Two matched samples of jejunum and terminal ileum were collected during organ procurement from transplant donors. Data were collected on age, sex, and BMI, and participants stratified as lean versus obese (BMI >30 kg/m²). Tissue samples from different regions of the human GI tract for LC-MS/MS were obtained from Addenbrooke’s Human Research Tissue Bank and the Cambridge Biorepository for Translational Medicine.

Samples were immediately placed in cold Leibovitz’s L-15 media (Thermo Scientific, Waltham, MA) and processed to the point of fixation or homogenized and stored at −70°C within 6 h.

FACS and RNA extraction from fixed human cells followed a modified version of the MARIS protocol (9). Intestine was rinsed in cold PBS and the muscular coat was removed. Diced mucosa was digested twice in 0.1% w/v collagenase XI (Sigma-Aldrich, St. Louis, MO) in Hanks’ Buffered Saline solution (HBSS) #9394 (Sigma-Aldrich) for 30 min each, shaking vigorously every 10 min. Supernatants were triturated, passed through a 50-μm filter and centrifuged at 300g. Pellets were resuspended in PBS and fixed in 4% w/v paraformaldehyde (PFA) at 4°C for 20 min. PFA-fixed cells were washed twice in nuclease free 1% w/v BSA in PBS, and if a FACS facility was not immediately available, they were suspended in 1% w/v BSA and 4% v/v RNAsin plus RNAse inhibitor (Promega, Fitchburg, WI) in PBS at 4°C overnight.

Cells were permeabilized with either a single 30-min incubation with 0.1% v/v Triton ×100 (Sigma-Aldrich) in 1% w/v BSA in PBS prior to antibody staining or by the addition of 0.1% w/v Saponin (Sigma-Aldrich) to solutions in all steps from this point until after the first wash postsecondary antibody staining, with identical results.

Primary antibody staining was for 1 h in 4% v/v RNAsin, 1% w/v BSA, 1% v/v goat anti-GLP-1 (sc7782; Santa Cruz, Dallas, TX), 2% v/v rabbit anti-chromogranin A (CHGA) (Ab15160; Abcam, Cambridge, U.K.), and 0.25% v/v rabbit anti-secretogranin 2 (SCG2) (Ab12241; Abcam) in PBS at 4°C. Cells were then washed twice in 1% w/v BSA and 1% v/v RNAsin, and secondary antibody staining was for 30 min in 4% v/v RNAsin, 1% w/v BSA, 0.2% v/v donkey anti-goat Alexa 555, and 0.2% v/v donkey anti-rabbit Alex 647 in PBS at 4°C. Cells were washed twice then suspended in 4% v/v RNAsin and 1% w/v BSA in PBS on ice for FACS.

Cell populations were sorted on a BD FACS ARIA III in the National Institute for Health Research (NIHR) Cambridge BRC Cell Phenotyping Hub or at Institut Cochin (Paris, France). Single cells positive for Alexa 647 but not Alexa 555 (i.e., CHGA/SCGA positive but GLP-1 negative) were classified as proglucagon negative (GCG⁻) enteroendocrine cells. Single cells positive for both Alexa 647 and Alexa 555 were classified as GCG⁺ enteroendocrine cells. At least 5,000 cells were collected for each positive population. Twenty thousand double-negative cells were collected as the negative (i.e., nonenteroendocrine) cell population. Cells were sorted into 2% v/v RNAsin in PBS at 4°C.

RNA was extracted using the Ambion RecoverAll Total Nucleic Acid Isolation Kit for FFPE (Ambion, Foster City, CA) with modifications to the protocol as below. The FACS-sorted cell suspension was centrifuged at 3,000g for 5 min at 4°C, and the pellet resuspended in 200 μL digestion buffer with 4 μL protease and incubated at 50°C for 3 h. The solution was then stored at −70°C for at least 12 h prior to further extraction. After thawing, RNA was extracted using the manufacturer’s protocol (including a DNase step), with the exception of performing 2× 60 μL elutions from the filter column in the final step.

The RNA solution was concentrated using a RNEasy MinElute cleanup kit (Qiagen, Hilden, Germany). RNA aliquots were diluted to 200 μL with nuclease-free water. The standard manufacturer’s protocol was followed, with the exception that 700 µL, not 500 µL, of 100% ethanol was added to the solution in step two to generate optimum binding conditions for the PFA-fragmented RNA. RNA concentration and quality was analyzed using an Agilent 2100 Bioanalyser (Agilent, Santa Clara, CA).

cDNA libraries were created using the Clontech SMARTer Stranded Total RNA-Seq Kit Pico Input Mammalian v1 (Takara Bio, Mountain View, CA). RNA input quantity was 5 ng, and the nonfragmentation protocol was used. The standard manufacturer’s protocol was followed, with the exception that 175 μL of AMPure beads was used for the final bead purification to ensure recovery of the small fragments of RNA arising from PFA fixation. Sixteen PCR cycles were used for amplification.

Fifty base single-end sequencing was performed using an Illumina HiSEQ 4000 at the Cancer Research UK Cambridge Institute Genomics Core.

Female NeuroD1-Cre/EYFP (mixed background, 3–10 generations backcrossed with C57BL/6) and GLU-Venus mice (C57BL/6) (6,7) aged 8–10 weeks were killed by cervical dislocation (n = 3 each). Diced mucosa from the proximal 10 cm of small intestine was digested twice in 0.1% w/v collagenase XI in HBSS at 37°C for 30 min each. Cells were pelleted by centrifugation at 300g for 5 min, triturated, and passed through a 50-μm filter. Cells were stained with DAPI (1 µg/mL) for 5 min at room temperature, washed twice, and sorted in HBSS on a FACSJazz sorter at the Cambridge NIHR BRC Cell Phenotyping Hub.

All positive cells, and 20,000 negative cells, were collected separately into aliquots of 500 μL of buffer RLT+ (Qiagen), with 143 mmol/L β-mercaptoethanol. RNA was extracted using a RNeasy Micro plus kit (Qiagen) and quantified using an Agilent 2100 Bioanalyser.

Two nanograms of each RNA were used for cDNA amplification by SPIA amplification using the Ovation RNAseq system V2 kit (NuGEN, Redwood City, CA). One microgram of cDNA was then fragmented to ∼200 bp by sonication (Diagenode, Liege, Belgium), and adaptors for the indexing were added using the Ovation Rapid DR multiplex 1–96 kit. Samples were pooled and concentrated together with a MinElute column (Qiagen) to reach a concentration of 10 nmol/L. Single-end 50 base sequencing was performed at the Cancer Research UK Cambridge Institute Genomics Core with an Illumina Hiseq4000.

Quality control and trimming of adaptors was performed using FastQC (10). Human sequenced transcripts were mapped to the human genome (GRCh37), and raw counts were generated using STAR v2.5.1. Mouse reads were aligned to the mouse genome (GRCm38) using TopHat 2.1.0, and raw counts were generated using Cufflinks 2.2.1 (11–13). Differential gene expression analysis was performed in RStudio using DESEQ2 (14). Gene annotation was pulled from the Ensembl data set held in BioMart (11). Receptor and ion channel lists were generated from the International Union of Basic and Clinical Pharmacology (IUPHAR)/British Pharmacological Society (BPS) “targets and families” list (15). Graphical output used ggplot2 and pheatmap in RStudio (16).

Mouse and human data sets were directly compared using only the 15,507 genes present in both data sets, not annotated as ribosomal, mitochondrial, or small nuclear, and described with one-to-one homology according to the Ensembl mouse-human homology data set (11). Genes with no one-to-one homology were analyzed separately. Normalized CPM (counts per million) were generated from the respective DESEQ2 models and compared for the human GCG⁺ population versus the murine GLU-Venus population and the human GCG⁻ population versus the murine NeuroD1 population. Linear models were generated of the log₁₀ CPM of the human versus murine data sets by a total least squares strategy, 99% CI calculated, and the outliers hand-searched for relevant genes.

Examining just the human samples, DESEQ2 models were generated for the following sets of jejunum samples: GCG⁺ versus negative, GCG⁻ versus negative, GCG⁺ versus GCG⁻, GCG⁺ lean versus obese, and GCG⁻ lean versus obese. Participant-paired DESEQ2 analyses were also performed comparing GCG⁺ and GCG⁻ populations from the jejunum and ileum of the two transplant donor participants, for whom there were matched jejunum and ileum samples. An adjusted P value of ≤0.1 was defined as the cutoff for statistical significance when examining for differential gene expression between populations.

Small pieces (∼2 × 2 mm, 15–45 mg) of mucosa from different regions of the human or mouse GI tract were homogenized in 250 μL of 6 mol/L guanidine hydrochloride (Sigma-Aldrich) with Lyzing MatrixD (MPbio) in a FastPrep-24 for 4 × 40 s at 6 ms⁻¹. Samples were stored at −70°C before further processing. Proteins were precipitated by adding 80% acetonitrile in water then centrifuged at 12,000g at 4°C for 5 min. The aqueous phase containing the peptides was collected, dried on a centrifugal vacuum concentrator, and stored at −70°C before analysis.

Samples were extracted using a Waters HLB μElution solid‐phase extraction plate (Waters, Milford, MA) after being resuspended in 500 μL 0.1% v/v formic acid in water as described previously and analyzed after reduction/alkylation (17). Human homogenates and mouse homogenates for interspecies comparison were analyzed using nanoflow-based separation and electrospray approaches on a Thermo Fisher Ultimate 3000 Nano LC system coupled to a Q Exactive Plus Orbitrap mass spectrometer (Thermo Scientific). High-flow separation for the longitudinal mouse analysis was done as previously described (17). Downstream analysis was performed using Peaks 8.0 software (Waterloo, Ontario, Canada) against the human and the mouse Swiss-Prot databases (downloaded 26 October 2017) (18), with a fixed cysteine carbamidomethylation and variable methionine oxidation, N-terminal acetylation, and pyro-glutamate and COOH-terminal amidation modifications. Manual searches were performed for other modifications. Peptides of interest were quantified by measuring peak areas for selected m/z ranges and retention times corresponding to the peptide sequences and normalized by tissue weight.

Human intestinal tissue pieces were digested, PFA fixed, and stained for CHGA and SCG2 as general markers for EECs and for GLP-1 as a marker of the EEC-subpopulation known as L-cells. By flow cytometry (Supplementary Fig. 1A–C), we collected pooled cell populations that were 1) positive for CHGA, SCG2, and GLP-1 (henceforth named GCG⁺), 2) positive for CHGA and SCG2 but negative for GLP-1 (henceforth named GCG⁻), and 3) negative for all three markers (i.e., nonendocrine lineage cells, henceforth named negative). The GCG⁺ (L-cell) population represented ∼0.2% of all single cells examined, and the ratio of GCG⁺ to GCG⁻ cells was ∼1:5.

From mice, we collected unfixed EEC populations from the upper small intestine of the mouse strain GLU-Venus (n = 3) to identify Gcg-expressing L-cells (Supplementary Fig. 1E–G) (7) and of NeuroD1-Cre/EYFP strain (6) (n = 3) to identify the total EEC population (Supplementary Fig. 1I–K). GLU-Venus positive cells represented ∼0.2% of singlets, and NeuroD1 positive cells, ∼0.6% of singlets.

RNA extracted from the purified fixed human cell populations had measured RNA integrity number (RIN) values of 2–3 (compared with >7 in the unfixed murine cells), with most RNA fragments being 25–500 bases in length (Supplementary Fig. 1D). The low RIN values of the human samples reflect the simultaneous fragmentation of ribosomal RNAs, but we predicted that the fragments were of lengths suitable for RNA sequencing using random primers and an rRNA depletion protocol. After RNA sequencing, a mean of 77% of reads from the human samples mapped to the human genome, compared with 86% of reads mapping to the murine genome in the mouse samples. The mean number of reads mapping uniquely to exons was 3.5 × 10⁶ (range 0.8 × 10⁶ to 8.8 × 10⁶) in the human samples, and 3.9 × 10⁶ (range 2.0 × 10⁶ to 5.7 × 10⁶) in murine samples.

In total, we obtained individual RNA sequencing data from GCG⁺, GCG⁻, and negative cells from each of 11 human jejunum samples and 2 human ileum samples. Principle component analysis of the top 500 differentially expressed genes in the jejunal samples separated EECs (GCG⁺ and GCG⁻) from negative cells on the first component, and GCG⁺ cells from GCG⁻ cells on the second component (Fig. 1A). Principle component analysis did not demonstrate clustering of samples by BMI of the donor. A heatmap of the top 500 differentially expressed genes (Fig. 1B) revealed clear transcriptomic differences between the GCG⁺, GCG⁻, and negative cells (14). A comparison between jejunal and ileal cell populations from the two matched donors is shown in Supplementary Fig. 2.

Human jejunal EEC populations expressed a wide range of hormonal transcripts (Fig. 2A, C, and E). As GLP-1 antibodies were used to purify the GCG⁺ cells, we were not surprised that the hormonal transcript showing the strongest differential expression between GCG⁺ and GCG⁻ cells was GCG itself (Fig. 2C). Consistent with previous findings in mice (3,19–21), human GCG⁺ cells also expressed a range of additional hormonal transcripts including GIP (glucose-dependent insulinotropic polypeptide), CCK (cholecystokinin), NTS (neurotensin), PYY, and SCT (secretin) as well as MLN (motilin), a hormone produced by human but not mouse (3,19–22). Compared with GCG⁺ cells, GCG⁻ cells had higher expression of SCT, CCK, NTS, MLN, GHRL (ghrelin), and SST (somatostatin), as well as TPH1, the enzyme responsible for serotonin biosynthesis in enterochromaffin cells. EECs also expressed the putative gut hormones UCN3 (urocortin 3), PCSK1N (ProSAAS), and NPW (neuropeptide W), as well as lower levels of RNAs encoding peptides not classically described as gut hormones, such as VGF, GHRH, and ADM.

Transcripts of ∼50 GPCRs were either enriched in EECs compared with negative cells, or expressed at >100 CPM in one or both EEC populations (Fig. 2B, D, and F). Multiple GPCRs previously implicated in postprandial gut hormone secretion in mice were highly expressed in human EECs, including the fat-sensing receptors FFAR1, FFAR2, FFAR3, FFAR4, and GPR119, the amino acid–sensing receptors CASR and GPR142, the butyrate- and isovalerate-sensing OR51E1 (23), and the bile acid receptor, GPBAR1. At least four orphan GPCRs were differentially expressed in human EECs, GPR148, GPR160, GPR173, and GPR179, hinting to as-yet-undescribed pathways that may control gut hormone secretion.

Human EECs expressed transcripts for a range of ion channel subunits (Supplementary Fig. 3), consistent with previous reports that murine L-cells and enterochromaffin cells are electrically active (24). Transcription factor profiling of human GCG⁺ and GCG⁻ cells is shown in Supplementary Fig. 3.

To compare the L-cell populations between humans and mice, we compared human jejunal GCG⁺ cells with murine upper small intestinal GLU-Venus cells (Fig. 3). Log-log plots of normalized gene expression indicated a strong correlation between the two species (R² = 0.73) (Fig. 4). Notable genes more highly expressed in human than mouse L-cells included GIP, CHGA, ASIC5, GIPR, GPR142, SCTR, PTH2R, CHRNA5, and OPRK1, whereas genes more highly expressed in mice included Gpr174, Gpr171, Ghr, Grpr, Ptger1, Cnr1, Insl5, Gpr22, and Ghrl.

A similar comparison was made between human jejunal GCG⁻ cells, representing the wider EEC population (although depleted of L-cells) and murine NeuroD1-positive cells, which similarly revealed a strong interspecies correlation (R² = 0.74) (Fig. 4). Data on transcription factors, GPCRs, ion channels, and hormones that were EEC-enriched in either species but excluded from the comparative analysis because they did not have annotated 1:1 orthologs between mouse and human are given in Supplementary Table 2 and notably highlight MLN and GPR148 as EEC-enriched transcripts in humans that are not found in mice.

Peptide extraction and LC-MS/MS protocols were optimized for maximum peptide retrieval and identification from fresh intestinal mucosal samples (Supplementary Fig. 4) and enabled reliable detection and sequencing of peptides up to 65 amino acids in length. In the first instance, we compared human jejunum with mouse mid–small intestine and assigned peptides to their parental proteins. This method identified known EEC prohormones, granins, and enteric neuronal signaling peptides, as well as peptides derived from a variety of housekeeping proteins that likely reflected the occurrence of some tissue damage/degradation prior to homogenization. Of the 463 and 705 different proteins matched in humans and mice, respectively, 234 were common between the two species and showed good correlation (R² = 0.54) (Fig. 5A). To identify candidate EEC-derived peptides, we restricted the analysis to peptides originating from genes that in the transcriptomic analysis showed a greater than fourfold higher expression in at least one EEC sample compared with the corresponding negative cells (Fig. 5B). Known gut hormone genes and members of the chromogranin family were mostly found to be common between mouse and human, but motilin and ghrelin were detected in human but not mouse jejunum. To search for novel candidate peptide hormones, we also examined the transcriptomic data for unannotated transcripts that had a base mean value >100 and were greater than 16-fold more highly expressed in EECs than control cells. This analysis identified MIR7–3HG (25), C1orf127, and C6orf141, but we were unable to detect corresponding peptides by LC-MS/MS.

We performed a longitudinal LC-MS/MS analysis of known bioactive peptides along the mouse and human GI tracts. Most EEC peptides were identifiable in their known bioactive forms, but as our method was not optimized for very small peptides like CCK-8, we used CCK_21-44 as a surrogate for CCK production. Peptides have been depicted in separate heatmaps for mouse and human (Fig. 6), separated according to their origin from EEC prohormones, granins, and non-EECs (likely reflecting enteric neural peptides). We observed longitudinal peptide profiles that broadly mirror historical immunostaining patterns (26) but additionally provide details of the exact peptide sequences and their posttranslational modifications.

By RNA sequencing of fixed, FACS-purified cells from the human gut, we report here the transcriptome of human L-cells and the wider EEC population and a between-species comparison showing a strong similarity with matching cells from the mouse. LC-MS/MS–based peptidomic analysis of the human and mouse gut revealed longitudinal gradients of a range of EEC peptides, including details of their exact sequences and posttranslational modifications.

To purify human EECs for transcriptomics, cells were first fixed, permeabilized, and antibody stained, and the RNA extraction and sequencing kits were only just technically capable of dealing with PFA-modified RNA. Nevertheless, the RNAseq-derived transcriptomes of human L-cells and GCG⁻ EECs mapped robustly onto the corresponding data from freshly purified matching murine EEC populations and the read depth was sufficient for the detection of low-abundance mRNAs, such as those encoding receptors and ion channels. Although we analyzed samples from 11 humans with varying BMI, we were unable to detect any effect of BMI on the EEC transcriptome. However, the study was not designed or powered to address the impact of BMI or diet on EECs, and further studies will be needed to examine this question.

GPCRs play key sensory roles in EECs and a number are under investigation as candidate drug targets for enhancing gut hormone secretion as a therapy for type 2 diabetes and obesity. The GPCR repertoire of human EECs largely mirrored their well-studied murine counterparts (8,27–29), including expression of receptors for amino acids (CASR, GPR142), triglyceride digestion products (FFAR1, FFAR4, GPR119), and bile acids (GPBAR1), as well as for hormones such as somatostatin (SSTR1, SSTR2, SSTR5), GIP (GIPR), and arginine vasopressin (AVPR1B). Interestingly, GPR142 was highly expressed in human EECs, supporting current studies looking to exploit its ability to stimulate both insulin and incretin hormone secretion (28).

Our optimized peptide extraction protocol combined with nano-LC-MS/MS analysis enabled identification of the exact peptide sequences biosynthesized in human and mouse intestinal mucosa, including posttranslational modifications, for peptides ranging from ∼8–10 to 65 amino acids in length. From the proglucagon gene, for example, we detected multiple processed and preprocessed products, including GRPP, oxyntomodulin, GLP-1_{7-36 amide}, GLP-1_7-37, GLP-1_1-37, IP_131-142, IP-GLP2, and GLP-2. Intact (pancreatic-type) glucagon was detected in samples from the mouse stomach but was undetectable in the remainder of the intestine and colon from both species, conflicting with recent suggestions that the small intestine secretes intact glucagon (30) but consistent with our recent finding that postprandial glucagon concentrations were not altered following gastric bypass surgery in lean subjects despite dramatic increases in GLP-1 (31). LC-MS/MS also identified some additional peptides encoded by EEC-enriched genes, including peptides derived from PCSK1N, chromogranins, and secretogranins. Whether any of these have specific physiological roles or are simply inactive by-products of enzymatic processing of the contents of secretory vesicles requires further evaluation.

Mapping of gut hormone production along the GI tract length has previously been performed by immunostaining or extraction/immunoassays for specific peptides (26,32). Many antibody-based methods, however, do not distinguish whether a prohormone was processed or unprocessed or posttranslationally modified. Our LC-MS/MS method provides a robust mirror of previous antibody-based maps of the GI tract, while additionally assigning an exact peptide sequence to each identified peptide, clearly distinguishing, for example, oxyntomodulin from glucagon and PYY_1-36 from PYY_3-36. Interestingly, we identified acylated as well as nonacylated ghrelin from the human jejunum despite our previous finding that plasma acylated ghrelin levels were undetectable in humans after total gastrectomy (31). We were surprised to find high levels of PYY_3-36 as well as PYY_1-36 in tissue homogenates, suggesting that dipeptidyl peptidases (DPPs) are active within L-cells, although GLP-1_{7-36 amide} was much more abundant than GLP-1_{9-36 amide}. Why GLP-1 but not PYY seems protected from DPP-mediated processing in L-cells, despite both peptides being located in the same vesicular pool (33), remains unclear.

The methods we describe here for performing RNA sequencing of rare cell populations and LC-MS/MS–based peptidomic analysis from human surgical tissue samples have wide potential applications beyond the study of the enteroendocrine system, including islet cell biology. Although comparison of the human and mouse EEC transcriptomes revealed strong global similarities between the two species, variation at the level of individual genes could have profound implications for the use of mice as a model species in drug development programs targeting specific receptors. Our mouse/human comparative data sets provide tools for assessing the validity of using mice as a model for investigating specific signaling pathways in humans, and the human EEC GPCR-ome can be used independently as a potential source of drug targets in the human enteroendocrine system. Longitudinal peptide mapping of the GI tract by LC-MS/MS is a key step toward understanding the metabolic benefits of gastric bypass surgery, as most bariatric procedures result in a shift in the location of nutrient digestion and absorption to more distal regions of the small intestine, with consequent stimulation of the more distal EEC population and release of their distinct profiles of peptide hormones. The results presented here should guide strategies to mimic gastric bypass surgery using injectable peptide mimetics or by targeting EEC-enriched receptors to mobilize endogenous gut hormones, which are highly topical challenges for industry and academia alike.

Acknowledgments. The authors would like to thank the surgical team in the Cambridge Oesophago-Gastric Centre in Cambridge and Sébastien Czernichow (Assistance Publique Hôpitaux de Paris, Georges Pompidou European Hospital, Paris, France) and Cyrille Ramond (Department of Endocrinology, Metabolism and Diabetes, INSERM U1016, Institut Cochin, Université Paris-Descartes, Paris, France), as well as the Cambridge Biorepository for Translational Medicine and the NIHR Cambridge Human Research Tissue Bank for assistance with the collection of donor tissue. FACS was supported by the Institut Cochin in Paris and the Cambridge NIHR BRC Cell Phenotyping Hub. RNA-sequencing was undertaken at the Cancer Research UK Cambridge Institute Genomics Core.

Funding. Metabolic Research Laboratories support was provided by the following core facilities: Disease Model Core, Genomics and Transcriptomics Core, Histology Core, Imaging Core, and NIHR BRC Core Biochemical Assay Laboratory (supported by the Medical Research Council [MRC_MC_UU_12012/5] and Wellcome Trust [100574/Z/12/Z]). G.P.R. received an Addenbrooke’s Charitable Trust/Evelyn Trust Cambridge Clinical Research Fellowship [16-69], an European Foundation for the Study of Diabetes project grant, and a Royal College of Surgeons Research Fellowship. S.G.G. is supported by a grant from the Biotechnology and Biological Sciences Research Council. Research in the laboratory of F.M.G. and F.R. is supported by the MRC (MRC_MC_UU_12012/3) and Wellcome Trust (106262/Z/14/Z and 106263/Z/14/Z) The MS instrument was funded by the MRC “Enhancing UK clinical research” grant (MR/M009041/1). P.R. was supported by a postdoctoral grant from Agence Nationale de la Recherche (Laboratoire d'Excellence Revive, Investissement d'Avenir, ANR-10-LABX-73). The laboratory of R.S. is supported by Agence Nationale de la Recherche (ANR-10-LABX-73) and the Bettencourt-Schueller Foundation. This work was partially supported by the following National Institutes of Health grants R01 DK100223-02 and R01 DK110614-01 (to A.L.).

Duality of Interest. F.M.G. is a paid consultant for and P.R. has (subsequent to his work on this project) taken up full-time employment with Kallyope (New York, NY). The laboratory of F.R. and F.M.G. hosts projects that receive funding from Medimmune. No other potential conflicts of interest relevant to this article were reported.

Author Contributions. G.P.R., P.L., P.R., R.S., R.H.H., F.R., and F.M.G. designed the study. Tissue handling and FACS were performed by G.P.R., P.L., P.R., and L.L.G. cDNA library production and bioinformatics analysis were performed by G.P.R., P.L., P.R., M.K.L.M., and B.L., with support from G.S.H.Y. and D.C. Mass spectrometry was performed by G.P.R., P.L., R.G.K., S.G.G., and E.L.M. NeuroD1 mice were generated by A.L. and H.J.L. The manuscript was written by G.P.R., F.R., and F.M.G. All authors had editorial oversight of the final manuscript version. F.R. and F.M.G. are the guarantors of this work and, as such, had full access to all the data in the study and take responsibility for the integrity of the data and the accuracy of the data analysis.

Data Availability. The mass spectrometry proteomics data have been deposited to the ProteomeXchange Consortium via the PRIDE partner repository with the data set identifiers PXD009788 (10.6019/PXD009788) and PXD009796 (10.6019/PXD009796) (see Vizcaíno JA, Csordas A, del-Toro N, et al. 2016 update of the PRIDE database and its related tools. Nucleic Acids Res 2016;44:D447–D456). RNA-seq data has been deposited in the NCBI GEO repository (human, GSE114853; mouse, GSE114913).

Prior Presentation. A non–peer-reviewed version of this article was submitted to the bioRxiv preprint server (doi: https://doi.org/10.1101/374579) on 23 July 2018.