Regulated and adaptive in vivo insulin secretion from islets only containing β-cells

Perez-Frances, Marta; Bru-Tari, Eva; Cohrs, Christian; Abate, Maria Valentina; van Gurp, Léon; Furuyama, Kenichiro; Speier, Stephan; Thorel, Fabrizio; Herrera, Pedro L.

doi:10.1038/s42255-024-01114-8

Regulated and adaptive in vivo insulin secretion from islets only containing β-cells

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Published: 21 August 2024

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Regulated and adaptive in vivo insulin secretion from islets only containing β-cells

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Abstract

Insulin-producing β-cells in pancreatic islets are regulated by systemic cues and, locally, by adjacent islet hormone-producing ‘non-β-cells’ (namely α-cells, δ-cells and γ-cells). Yet whether the non-β-cells are required for accurate insulin secretion is unclear. Here, we studied mice in which adult islets are exclusively composed of β-cells and human pseudoislets containing only primary β-cells. Mice lacking non-β-cells had optimal blood glucose regulation, enhanced glucose tolerance, insulin sensitivity and restricted body weight gain under a high-fat diet. The insulin secretion dynamics in islets composed of only β-cells was comparable to that in intact islets. Similarly, human β-cell pseudoislets retained the glucose-regulated mitochondrial respiration, insulin secretion and exendin-4 responses of entire islets. The findings indicate that non-β-cells are dispensable for blood glucose homeostasis and β-cell function. These results support efforts aimed at developing diabetes treatments by generating β-like clusters devoid of non-β-cells, such as from pluripotent stem cells differentiated in vitro or by reprograming non-β-cells into insulin producers in situ.

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Main

Glucose homeostasis is the maintenance of blood glucose (glycaemia) levels within a narrow range to meet the body’s fluctuating metabolic demands. The rapid and delicate adjustment of glycaemia involves a complex interplay of hormones and neuropeptides that are released into the blood from multiple organs, including the brain, liver, intestine, adipose tissue, muscle and pancreas.

Pancreatic islets have an essential role in glucose homeostasis through the secretion of various hormones, particularly insulin, which stimulates blood glucose uptake from peripheral tissues. Insulin released from β-cells is tightly regulated by circulating glucose levels but also by stimuli originating from islet α-cells, δ-cells and γ-cells¹. For example, glucagon (GCG) produced by α-cells is a major glucose counter-regulatory hormone through its actions in modulating β-cell secretory activity². Indeed, blocking GCG signalling by inactivating the GCG receptor (GCGR) or using GCGR-neutralizing antibodies reduces insulin release^2,3. Moreover, corticotropin-releasing hormone and acetylcholine, both secreted from α-cells, can stimulate insulin secretion under certain physiological conditions^4,5. Glucose-induced somatostatin (SST) secretion by δ-cells is also a powerful inhibitor of both GCG and insulin secretion⁶. Lastly, the pancreatic polypeptide (PPY) secreted from γ-cells can also reduce the secretion of insulin^7,8. Collectively, these results strongly suggest that neighboring islet α-cells, δ-cells and- γ-cells have an important role in controlling insulin secretion from β-cells.

We have previously shown that islet non-β-cells have the intrinsic capacity of being converted to insulin-producing β-like cells under certain conditions, such as, for example, upon the loss of β-cells, which is a feature of diabetes mellitus^{9,10,11,12,13,14}. Observing such plasticity in endogenous islet α-cells, δ-cells and γ-cells raises the possibility of exploiting this property to treat diabetes. This therapeutic strategy will result in islets that exclusively contain surrogate insulin-producing cells, and it is unknown whether interfering with local intra-islet signalling will impact insulin secretion and blood glucose homeostasis in vivo. Consequently, we developed a mouse model that selectively and simultaneously removed α-cells, δ-cells and γ-cells while preserving an intact β-cell mass. In addition, we studied monotypic pseudoislets containing human primary β-cells only. These approaches enabled the exploration of how regulated insulin secretion and blood glucose homeostasis are affected in islets composed exclusively of β-cells.

Results

Generation of a mouse model of islet non-β-cell loss

To determine the necessity of islet non-β-cells in controlling glucose homeostasis and β-cell function, we generated triply transgenic mice allowing the inducible diphtheria toxin (DT)-mediated ablation of adult α-cells, δ-cells and γ-cells (‘non-βDTR’ mice). DT receptor (DTR) expression in islet cells was driven by the Gcg, Sst and Ppy promoters. The non-βDTR mice were obtained by breeding the Glu-DTR (transgenic)¹⁵ and Ppy-DTR (knock-in)¹⁴ lines to a new Sst-DTR knock-in line. Sst-DTR mice were generated using CRISPR technology to replace the coding sequence of the Sst gene with the DTR coding region (Fig. 1a). The knock-in Sst-DTR and Ppy-DTR alleles were bred to hemizygosity in non-βDTR mice (Fig. 1b) to secure both hormone and DTR expression in δ-cells and γ-cells, respectively (Fig. 1c).

**Fig. 1: Generation and characterization of transgenic mice for the simultaneous ablation of islet α-cells, δ-cells and γ-cells.**

Non-βDTR mice were given DT at 2 months of age. DT-treated non-βDTR mice (hereafter, ‘β-only’ mice) showed a >99% reduction in α-cell, δ-cell and γ-cell numbers 4 weeks post ablation (wpa; that is, at 3 months of age) compared with untreated mice (GCG⁺ > 99.9%, SST⁺ > 99.9%, PPY⁺ > 99.9% ablation efficiency; Fig. 1d,e). Islet Gcg, Sst and Ppy mRNA levels were reduced to 0.4%, 0.2% and 0.5%, respectively (Fig. 1f). The near total loss of α-cells, δ-cells and γ-cells was maintained in mice approaching 1 year of age (40 wpa), with no evidence of non-β-cell regeneration (Fig. 1d,e and Extended Data Fig. 1). Pancreatic insulin content was unaltered in β-only mice (Fig. 1g and Extended Data Fig. 1). In conclusion, the non-βDTR line allows the selective, inducible and efficient ablation of α-cells, δ-cells and γ-cells and thus represents a unique model to study the regulatory properties of pancreatic islets composed exclusively of β-cells.

Proper glucose homeostasis in β-only mice

To examine the effect of non-β-cell loss on blood glucose regulation, male and female β-only mice were analysed longitudinally for a period of 40 wpa. These mice were healthy, with normal glycaemia, body weight and body composition (Fig. 2a and Extended Data Figs. 2 and 3). Yet there was a transient reduction in glycaemia and body weight at 2 wpa, coincident with the DT-mediated ablation of gut SST-expressing δ-cells (Extended Data Figs. 2 and 3). However, intestinal δ-cells were restored and SST circulating levels were back to normal by 30 days post ablation (dpa) (Extended Data Fig. 2). Of note, this transient drop in glycaemia and body weight was also observed after the ablation of δ-cells only, but not after the loss of either α-cells or γ-cells separately (Extended Data Fig. 4 and Supplementary Table 1). To avoid any confounding effects caused by this transient phenotype, all subsequent experiments were performed using β-only mice at 4 wpa or later time points.

**Fig. 2: Optimal blood glucose homeostasis in mice whose islets comprise β-cells only.**

Hypothalamic Sst-expressing neurons probably exert an orexigenic function by controlling feeding and physical behaviours^16,17,18,19. After DT treatment, the ablation of SST⁺ neurons was only partial in β-only mice, which may explain the unaltered food intake and locomotor activity (Extended Data Fig. 2). β-only mice were normoglycaemic under random-fed conditions and after short and prolonged fasting despite the drastic reduction in pancreatic GCG (Figs. 2a and 3a). Indeed, the moderate decrease in circulating GCG, which was already reported after α-cell ablation^15,20, as well as the normal levels of plasma counter-regulatory hormones (cortisol, growth hormone and epinephrine) probably prevented hypoglycaemia (Fig. 3b–f)^3,21. In addition, liver-induced glucose mobilization, pyruvate and lactate levels, glycogen storage as well as the mRNA levels of gluconeogenic enzymes were comparably regulated in β-only and controls (that is, untreated non-βDTR mice) after a prolonged 16-h fasting challenge (Fig. 3g–k). These observations support previous reports indicating that the counter-regulatory responses to hypoglycaemia are maintained after extreme α-cell loss³.

**Fig. 3: The ablation of pancreatic α-cells has no effect on GCG-mediated hepatic function.**

We then assessed glucose tolerance in β-only males and females. Oral, but not intraperitoneal glucose tolerance was improved after DT treatment, suggesting that non-β-cell ablation leads to an enhanced incretin effect (Fig. 2b–d and Extended Data Fig. 3). Notably, circulating GLP-1 levels and glucose-stimulated insulin secretion were increased in β-only mice after glucose gavage (Fig. 2e,f and Extended Data Fig. 3). DT-treated mice also exhibited improved insulin sensitivity correlating with increased glucose uptake in white adipose tissue (WAT; Fig. 2g,h and Extended Data Fig. 3). Enhanced insulin sensitivity was further confirmed with a hyperinsulinemic–euglycaemic clamp: β-only mice showed increased glucose infusion rate, enhanced hepatic insulin sensitivity and higher glucose absorption in WAT (Extended Data Fig. 5). Metabolic cages were then used to further characterize the metabolic status of β-only mice. Although energy expenditure was similar during the dark phase, a slight increase during the light period was observed in DT-treated mice (Fig. 2i). Interestingly, the subtle but significant decrease in the respiratory exchange ratio during the day phase indicated that β-only mice rely more on lipid than carbohydrate catabolism (Fig. 2j). The observed increase in glucose uptake in WAT, together with the higher lipid catabolism, suggests that adipose tissue metabolism is enhanced in β-only mice. Altogether, these results revealed that the absence of α-cells, δ-cells and γ-cells does not lead to detrimental effects on glucose homeostasis. Instead, several metabolic parameters are improved.

Improved glucose homeostasis in β-only mice on a high-fat diet

As the ablation of islet non-β-cells had no deleterious effects on glucose regulation under homeostatic conditions, we next investigated how the metabolic stress induced by a high-fat diet (HFD) affects β-only mice relative to controls. To this end, we devised four experimental groups of mice treated with or without DT and raised on either a chow or HFD (60% fat) regimen. High-fat or control diets were given to 3-month-old males (4 wpa) for 24 weeks (Fig. 4a). Strikingly, DT-treated non-βDTR animals showed a restricted body weight gain and limited increase in fat mass under HFD compared to challenged control mice (Fig. 4b,c). Importantly, food intake quantities were equal in all experimental groups (Extended Data Fig. 6). Fasting and random-fed glycaemia in the HFD group were higher in mice with intact islets relative to β-only animals (Fig. 4d and Extended Data Fig. 6). In addition, β-only mice exhibited better glucose tolerance than controls, which became glucose-intolerant (Fig. 4e and Extended Data Fig. 6). Of note, oral glucose tolerance in β-only mice under a HFD was like that of control mice under a chow diet (Fig. 4e). The control mice also manifested higher basal and glucose-stimulated insulin secretion than β-only mice under the HFD regimen. This suggests that HFD treatment triggers insulin resistance in control but not in β-only mice (Fig. 4f and Extended Data Fig. 6). This was confirmed by the worsened insulin sensitivity in HFD-raised control mice (Fig. 4g). By contrast, β-only mice challenged with HFD retained the improved insulin sensitivity first observed under homeostatic conditions (Fig. 4g). Thus, the combined loss of GCG-expressing, SST-expressing and PPY-expressing cells limits body weight gain rates under HFD. This can be explained, at least in part, by the enhanced insulin sensitivity acquired after non-β-cell ablation.

**Fig. 4: Restricted body weight gain and better glucose homeostasis in β-only mice under HFD.**

Islet non-β-cell loss drives the phenotype of β-only mice

The significant decrease in the number of SST-expressing neurons in the brain upon DT-mediated non-β-cell ablation (Extended Data Fig. 2) could impact the β-only phenotype in vivo. Yet lowering the DT dosage (three injections of 5 ng of DT) significantly spared SST⁺ neurons without reducing the cell ablation efficiency in pancreatic islets (Extended Data Fig. 7). In the stomach, the SST-producing δ-cells were ablated at 15 dpa but reconstituted 2 weeks later, as in mice treated with the highest DT dose. Mice injected with 5 ng of DT did not display a sharp transient drop in body weight or glycaemia at 15 dpa (Extended Data Fig. 7), suggesting involvement of the SST-producing neurons in the transient phenotype observed with the high DT dosage. Interestingly, at 30 dpa, β-only mice treated with 5 ng of DT had improved oral glucose tolerance, glucose-stimulated insulin secretion and insulin sensitivity, similar to mice treated with a high DT dosage (Extended Data Fig. 7). Thus, the phenotype of β-only mice from 1 month post ablation is determined by the lack of islet non-β-cells.

β-only islets have a normal insulin secretion profile

To evaluate the intrinsic capacity of β-only islets to regulate insulin secretion without the influence of peripheral tissues, we assessed the glucose-stimulated insulin secretion response in perfused pancreatic slices²² (Fig. 5a). Pancreatic slices from β-only mice had the same insulin secretion pattern as those containing intact islets from controls (Fig. 5b and Extended Data Fig. 8). In addition, a normal glucose-stimulated insulin secretion profile was also observed in islets isolated from β-only mice (Fig. 5c,d and Extended Data Fig. 8). These results revealed that the biphasic insulin secretion profile is conserved in islets exclusively composed of β-cells. Moreover, the potentiation of glucose-stimulated insulin secretion by exendin-4 (Ex-4, a GLP-1 agonist) was similar in isolated intact and β-only islets (Fig. 5e and Extended Data Fig. 8). Furthermore, β-only and control islets displayed the same mitochondrial respiratory capacity to increase the oxygen consumption rate (OCR) in response to glucose, with similar basal and maximal OCRs (Fig. 5f and Extended Data Fig. 8). Thus, maintenance of the β-cell secretory response correlates with the capacity to effectively engage oxidative phosphorylation for glucose oxidation in the absence of islet α-cells, δ-cells and γ-cells. The regular β-cell function in β-only mice was further supported by the unaltered gene expression and identity of β-cells under fasting or refed conditions (Extended Data Fig. 9).

**Fig. 5: Monotypic β-only islets have normal dynamic insulin secretion and islet respirometry.**

Next, we wondered whether islets containing only β-cells could enhance their secretory capacity under pathophysiological conditions, such as an extreme insulin demand. For this purpose, the insulin receptor antagonist S961 (ref. ¹²) was dispensed using an osmotic pump to impose chronic hyperglycaemia (around 30 mM) in control and β-only mice. Both groups behaved similarly and became overtly hyperglycaemic (Fig. 6a) and drastically increased their insulin secretion levels (Fig. 6b). Interestingly, the S961-induced β-cell proliferation was enhanced in β-only islets as compared to controls (Fig. 6c,d). Altogether, these results indicate that β-cell nutrient sensing and secretion are appropriately regulated under physiological and extreme insulin needs in mouse islets lacking α-cells, δ-cells and γ-cells.

**Fig. 6: Monotypic β-only islets have a normal response to extreme insulin demand.**

Human β-cell pseudoislets display optimal insulin secretion

To assess whether human β-cells also maintain their glucose sensing and insulin secretory capacities in the absence of α-cells, δ-cells and γ-cells, we generated human ‘islet-like’ cell clusters, termed pseudoislets, composed of either all the islet cell types (‘control pseudoislets’) or only fluorescence-activated cell sorting (FACS)-sorted β-cells (monotypic ‘β-pseudoislets’; Fig. 7a and Extended Data Fig. 10). A sharp reduction in GCG, SST and PPY mRNAs, but not INS mRNA, was observed in monotypic β-pseudoislets compared with control pseudoislets (Fig. 7b). Accordingly, GCG⁺, SST⁺ and PPY⁺ cells were not detectable in β-pseudoislets (Fig. 7c).

**Fig. 7: Human monotypic β-pseudoislets maintain glucose-stimulated insulin secretion and islet respirometry.**

Monotypic β-pseudoislets showed glucose-regulated insulin secretion, with levels similar to control pseudoislets at basal and stimulatory glucose concentrations (Fig. 7d). When further challenged with Ex-4, β-pseudoislets secreted more insulin than control pseudoislets (Fig. 7d), indicating a potentiation of the incretin response in the absence of α-cells, δ-cells and γ-cells. Similar results were obtained when assessing the stimulatory index (Extended Data Fig. 10). Like mouse β-only islets, human β-pseudoislets showed no significant differences in islet respirometry parameters compared to control pseudoislets (Fig. 7e and Extended Data Fig. 10). Thus, glucose-stimulated insulin secretion from human β-pseudoislets is closely correlated with their capacity to increase mitochondrial respiration in response to glucose (Fig. 7d,e and Extended Data Fig. 10). Altogether, these results indicate that human β-cells, like mouse β-cells, can sense glucose and secrete insulin in a regulated manner in the absence of α-cells, δ-cells and γ-cells.

Discussion

We describe a mouse model in which the adult pancreatic islets are exclusively made up of β-cells. The near total loss of non-β-cells in these mice does not affect their viability, motor and feeding behaviour, body weight or blood glucose homeostasis (fasting and random fed). This correlates with—and could be explained, at least in part by—the persistence of circulating SST and GCG after non-β-cell ablation. The modest decrease in glucagonaemia, which was previously described in mice lacking α-cells only^15,20, along with the preserved counter-regulatory actions of cortisol, epinephrine and/or growth hormone, probably prevent mild hypoglycaemia, as reported in mice with constitutive and complete GCG signalling abrogation^3,21. We could not assess blood PPY levels owing to the absence of reliable commercial kits, yet the fact that PPY knockout mice remain normoglycaemic in both homeostatic¹⁴ and HFD²³ conditions suggests that PPY is dispensable for blood glucose homeostasis. We also evaluated ex vivo the intrinsic capacity of islets devoid of α-cells, δ-cells and γ-cells to secrete insulin in response to glucose independently of the influence of peripheral tissues. Surprisingly, we found that pancreatic slices and isolated islets composed exclusively of β-cells exhibit insulin secretion dynamics similar to that of intact islets, with preserved first and second secretion phases upon glucose stimulation. This correlates with the transcriptomic and mitochondrial respiration analyses, which did not show major changes in β-cell identity and glucose metabolism.

Our results reveal an unexpected consistent improvement of insulin sensitivity and glucose tolerance in β-only mice of both genders. Coincidentally, although plasmatic GCG levels were moderately reduced after non-β-cell ablation, improved glucose tolerance associated with increased GLP-1 levels, better insulin sensitivity and restricted HFD-induced weight gain were also previously reported under extreme conditions of GCG signalling blockade³ (GCGR KO and GCGR-neutralizing antibody treatment).

Single-islet cell-type ablation (either α-cells, δ-cells or γ-cells; Supplementary Table 1) did not fully recapitulate the metabolic phenotype of β-only mice. The α-cell or γ-cell ablated mice did not exhibit an obvious metabolic phenotype, as previously shown^14,15. However, the absence of δ-cells led to a mild reduction of blood glucose levels (Extended Data Fig. 4), as it was previously shown in a similar mouse model of δ-cell ablation²⁴ and in Sst²⁵ or Hhex²⁶ null mice. The defects in β-cell function and blood glucose homeostasis associated with the absence of δ-cells are somehow compensated by the simultaneous removal of α-cells and γ-cells in β-only mice. We thus reason that the combined loss of all non-β cells may imbalance systemic hormone signalling (that is, the insulin/GCG ratio and GLP-1 levels, among others), triggering compensatory or adaptive mechanisms in peripheral organs such as the liver and WAT, which may explain the observed improved insulin sensitivity and fatty acid metabolism. The increased GLP-1 levels triggered by non-β-cell loss may participate in the phenotype of β-only mice under homeostatic and HFD conditions, as this intestinal incretin is an important regulator of blood glucose homeostasis through potentiation of glucose-stimulated insulin secretion^27,28,29, suppression of hepatic gluconeogenesis or glycogenolysis and of GCG secretion, satiety stimulation and improvement of insulin sensitivity^{27,28,29,30,31}. In addition, GLP-1 receptor agonists enhance insulin sensitivity in hepatic and adipose tissues and reduce obesity in diabetic animals and humans^{32,33,34,35,36}. Of note, the improved insulin sensitivity in β-only mice might be a result of the slightly lower basal insulin secretion observed in vivo after removal of the three islet cell types. This subtle decrease in basal insulin secretion may trigger better insulin sensitivity as an adaptive phenomenon. However, defining the precise contribution of each peripheral organ in the phenotype of β-only mice is difficult owing to the dynamic and complex interplay between the different tissues involved in glucose homeostasis and lipid metabolism. Overall, intra-islet interactions are superimposed to inputs from peripheral tissues and integrated within the islet network to minutely regulate the β-cell secretory activity.

The ability of β-cells to increase their secretion capacity in response to incretin potentiators or extreme insulin demand, such as GLP-1 receptor agonist or an insulin receptor blockade, was maintained in β-only mice. These observations were repeated with human β-cells, whereby the glucose-stimulated insulin secretion and the mitochondrial respiration capacity were preserved in β-pseudoislets. Interestingly, it has been postulated that GLP-1 secreted by human α-cells is required for regulated and synchronous insulin secretion from β-cells^37,38, yet here we show that human β-only pseudoislets maintain the incretin-stimulated insulin secretion like pseudoislets composed of all islet cell types.

Although α-cells, δ-cells and γ-cells unequivocally participate in the regulation of β-cell function, it is astonishing that both murine and human islets maintain proper insulin secretion in their absence. This optimal glucose-regulated insulin secretion strongly suggests that connectivity and communication of β-cells among themselves is crucial whereas the heterologous interactions between β-cells and non-β-cells are not. β-cells are functionally coupled through gap junctions among themselves and with non-β-cells within islets^39,40,41. Electrical coupling between β-cells is critical to ensure proper insulin secretion^42,43. Insulin release defects upon disruption of the gap junction connexin 36 illustrate the importance of the electrical coupling between β-cells for their synchronization, controlled intracellular Ca²⁺ oscillations and proper insulin secretory activity^42,43,44. The genetic or pharmacological inhibition of connexin 36 causes the loss of oscillatory insulin secretion^44,45. Reaggregation of purified isolated primary human β-cells in cell clusters devoid of α-cells, δ-cells and γ-cells restores glucose-stimulated insulin secretion as compared to dispersed cells^13,46, supporting the notion that β-cell connectivity is key for regulated secretion activity in different species. In this context, human islet α-cells, δ-cells and γ-cells are intermingled among β-cells (which represent 50% of the islet cell mass), implying that most of the β-cells physically interact with non-β-cells^47,48,49. Conversely, in mouse islets, non-β-cells are mainly located at the islet periphery surrounding a central core of β-cells (representing 75% of the islet mass), an architecture that favours homotypic associations between β-cells over β-cell–non-β-cell interactions^48,50. The variable proportions and spatial distribution of the different islet cell types across species, together with the non-β-cell ablation data reported here, suggest that β-cell–non-β-cell direct interactions are not crucial to ensure properly regulated insulin secretion, contrary to what was thought so far.

Our results reveal that non-β-cells, when concomitantly lost, do not appear to be essential to ensure β-cell function in homeostatic or stress conditions, such as extreme insulin demand. Therefore, one wonders why adult pancreatic islets have α-cells, δ-cells and γ-cells. One possibility is that these cells had essential functions during evolution, but became somewhat ‘redundant’ as evolution progressed. For instance, GCG-expressing α-cells may have evolved as part of an essential counter-regulatory mechanism to cope with long periods of starvation and energy deficit. However, the presence of alternative counter-regulatory hormones could have attenuated the requirement of α-cells through evolution. Still, the lack of δ-cells impacts the threshold for glucose-stimulated insulin release²⁴, suggesting that the absence of this single cell type cannot be compensated, unless all non-β-cells are simultaneously depleted. Alternatively, or in addition, α-cells, δ-cells and γ-cells may have a direct role as supporting cells during embryonic development and perinatal maturation of β-cells^51,52. In line with this notion, a previous study showed that ablation of embryonic SST-expressing cells results in increased insulin content and excessive insulin release leading to severe hypoglycaemia and neonatal death⁵³. Yet other reports do not support a developmental role for embryonic δ-cells on β-cell maturation^52,54. Depletion of Ppy-expressing cells in mouse embryos led to a significant reduction in pancreatic insulin-containing and SST-containing cells, suggesting that the presence of γ-cells is crucial for β-cell and δ-cell differentiation^55,56. Likewise, GCG signalling was also shown to be critical for proper islet development and maturation⁵⁷.

Although defects in β-cell function and identity are clearly associated with diabetes, mounting evidence supports that the activity of non-β-cells is compromised in this condition. Although it is not clear how non-β-cells precisely contribute to disease progression and insulin secretion defects, our findings support that the absence of dysfunctional non-β-cells or strategies aimed at abrogating aberrant signalling from these cells would confer beneficial therapeutic effects in diabetes^11,58,59,60. It has been shown that α-cell dysfunction occurs at early stages of islet autoimmunity, before diabetes onset^61,62,63. Ongoing clinical trials are exploring the effect of GCGR antagonists on the hyperglucagonaemia typical of diabetic patients^64,65,66,67. Interestingly, insufficient secretion of GCG in response to hypoglycaemia in type 1 diabetes increases the risk of hypoglycaemic episodes under insulin therapy^68,69. In diabetic rodents, restoration of GCG levels during hypoglycaemia was described upon administration of SST receptor antagonists^70,71, suggesting that perturbed SST secretion could have a role in the absence of counter-regulatory response in diabetes^72,73.

At present, multiple therapeutic strategies are aimed at generating, either in vitro or in situ, insulin-producing β-like cells^74,75. The preserved glucose-stimulated insulin secretion in pancreatic islets made exclusively of β-cells, which is also found in aged mice and human cells, suggests that non-β-cells are dispensable for β-cell function. This supports current efforts aimed at generating functional surrogate β-like cells from stem cells⁷⁶, with particular attention to establishing adequate β-cell identity and cellular connectivity. These observations also clarify concerns about the decreased non-β-cell mass in situations whereby massive non-β-cell recruitment into insulin production and secretion was achieved to treat diabetes^74,77,78.

Methods

Animals

To generate the Sst-DTR knock-in mice, we used a CRISPR ribonucleoprotein complex containing the Cas9 protein along with the following two gRNAs: 5′-CAGGGCGCACTGGAGACGGC-3′ and 5′-ACAACAATATTAAAGCTAAC-3′ to target the SST locus. The donor plasmid (pBluescript II SK+) contained the DTR sequence flanked by a 2 kb right homology arm (upstream of the ATG in the Sst locus) and a 2 kb left homology arm (downstream of the STOP codon in the Sst locus). The ribonucleoprotein complex was co-injected with the donor plasmid in one-cell embryos. To generate this transgenic mouse model, the Sst-DTR transgene was combined with the previously described Gcg-DTR and Ppy-DTR transgenes. The non-β-DTR mice had a mixed genetic background.

Mice were housed in open cages, with densities varying depending on the size of the cage, in accordance with the Swiss regulation (Cage type S to L, Charles River). Cages were enriched with bedding, nestlet and a mouse house. Temperature and humidity in the housing room were maintained at 20–24 °C and 30–70%, respectively. The day–night cycles were programmed by alternating 12 h day and 12 h night. Animals received food and tap water ad libitum. Both male and female mice were used for experiments. Animals were randomly allocated to control or treatment groups. The study followed all ethical regulations regarding animal experimentation, and all experiments were performed under the guidelines of the Direction General de la Santé du Canton de Genève (license numbers GE/111/17, GE/121/17 and GE15820).

DT and S961 treatment

DT (Sigma-Aldrich) was injected intraperitoneally (126 ng of DT per injection on days 0, 1 and 2, or 5 ng of DT per injection on days 0, 3 and 6) to 2-month-old mice. S961 (Novo Nordisk) was given by ALZET osmotic pumps implanted subcutaneously (40 nmol per week).

Human islets and generation of human pseudoislets

All studies involving samples of human tissues were approved by the ethical committee of the University of Geneva. Human pancreatic islets were obtained from the Geneva University Hospital (Geneva, Switzerland), from the National Institute of Diabetes and Digestive and Kidney Diseases (NIDDK)-funded Integrated Islet Distribution Program (IIDP) at Beckman Research Institute of City of Hope (Duarte, CA, USA) and from the University of Alberta Diabetes Institute IsletCore (Edmonton, Alberta, Canada). All donors’ families gave informed consent for the use of pancreatic tissue in research. Subjects were de-identified at the source of organ procurement, whereby samples were assigned a unique identifier or RRID to ensure privacy. Donors' unique identifiers and basic metabolic details are described in Supplementary Table 4.

Upon arrival, islets were cultured overnight in fresh CMRL 1066 media (11530-037, Gibco) at 37 °C and 5% CO₂. Dissociation of human islets and staining with cell-surface antibodies to purify β-cells was performed as described previously^13,79. Stained cells were sorted on a Moflo Astrios (Beckman Coulter) system. Single viable islet cells were gated by forward-scatter, side-scatter and pulse-width parameters and by negative staining for DAPI (Invitrogen, D1306) to remove doublets and dead cells. For the formation of pseudoislets, agarose structures with spherical microwells were obtained by using a micro-mold (3D Petri Dish, Microtissues) and then used to promote self-assembly of the cells in a density of 1,000 cells per pseudoislet. Every other day, the culture media was changed. Experiments were performed 7 days after culture. Pseudoislet morphology and cell composition were evaluated by immunostaining and quantitative PCR with reverse transcription (RT–qPCR), as detailed below.

Islet isolation, FACS and RNA extraction

Islets were isolated from previously reported Insulin-mCherry mice, whose insulin-producing cells constitutively express mCherry¹². Cell sorting using FACS was performed as described in previous works^10,12,14 using a Moflo Astrios (Beckman Coutler) system with Summit v.6.2 (Beckman Coulter) software. Kaluza Analysis v.2.0 (Beckman Coulter) software was used for subsequent analyses. Islets were frozen in RLT buffer (Qiagen) with β-mercaptoethanol and stored at −80 °C before being processed for RNA extraction. RNA extraction from islets was performed using the Qiagen RNeasy Micro Kit. RNA extraction from tissue (duodenum, brain or liver) was performed using the Qiagen RNeasy Plus Universal Mini Kit.

RT–qPCR

Complementary DNA (cDNA) of total mouse islets, human pseudoislets, duodenum, liver and/or brain fractions was generated using the Qiagen QuantiTect Reverse Transcription Kit. qPCR reactions were performed using the appropriate primer mixes for each gene as well as the Express SyBr GreenER kit (Invitrogen, 100001652). We used the CorbettRobotics4 robot, and the PCR reaction was completed in the CorbettResearch6000 series cycler using a 40 cycles program. Normalization and analysis of the data were done with the RT–PCR analysis_macro v.1.1 (the Genomic Platform, University of Geneva) using two normalization genes (Gapdh and β-actin). Samples were run in triplicate. For human pseudoislets, biological duplicates of each sample were run in triplicate. Expression levels were normalized to RN18S. Primer sequences are shown in Supplementary Table 2.

Bulk RNA sequencing

β-cells were FACS-sorted from 1-month post-ablation and control mice, either under fasting or fasting plus 2 h refed condition. Islets were isolated and dissociated as described above. RNA was extracted as described above and assessed for quality by an Agilent bioanalyser before library generation and sequencing. Library preparation, RNA sequencing and quality controls were performed in the Genomics Core Facility of the University of Geneva. Reverse transcription and cDNA amplification were performed using the SMARTer Ultra Low RNA Kit (Clontech). cDNA libraries were prepared using Nextera XT DNA Sample Preparation Kit (Illumina) and sequenced on an Illumina HiSeq4000 platform with single-end 100-bp reads.

Analyses were performed following previously established pipelines¹⁴. All sequencing data were uploaded to and aligned on the Galaxy project⁸⁰ against Ensembl reference genome GRCm38.p6 (release 100) using STAR version 2.7.2b⁸¹ in two-pass mapping mode. Aligned data were counted using HTSeq v.0.9.1 (ref. ⁸²) in union mode. Analyses were performed in a pairwise manner between the four conditions analysed using DESeq2 v.1.28.1 (ref. ⁸³). For each pairwise comparison, genes were discarded if they had fewer than five counts per sample on average. After calculating differential expression between groups, log₂(fold changes) were shrunken using the normal estimator⁸³. Genes were considered to be differentially expressed if the absolute shrunken log₂(fold changes) were ≥1 and adjusted P values were ≤0.05.

A previously generated β-ID gene list⁷⁹ was used to identify possible changes in identity and gene expression in β-cells after non-β-cell ablation.

Glucose tolerance test

Mice were fasted for 16 h before starting the experiments. Intraperitoneal or oral glucose tolerance tests were performed as previously described⁹. A 20% glucose solution was injected intraperitoneally or through gavage to fasted mice relative to their body weight. Glycaemia was measured before the injection and 15, 30, 60, 90 and 120 min after glucose administration.

Insulin tolerance test

Mice were intraperitoneally injected with insulin (0.5 U kg⁻¹ or 0.4 U kg⁻¹ for the HFD experiment; Actrapid, Novo Nordisk) after 5 h of fasting. Glycaemia was measured before and 20, 40 and 60 min after injection.

Tissue protein extracts

Pancreatic or intestinal tissues were homogenized in acid–ethanol solution (74% ethanol, 1.4% HCl), then sonicated and centrifuged. The supernatant was collected and used for the immunoassay experiments, which were performed following the manufacturer’s instructions (Mercodia Ultrasensitive Mouse Insulin ELISA 10-1249-01; Mercodia Glucagon ELISA 10-1281-01).

Brain tissue was homogenized in a lysis buffer containing 10× Cell Lysis Buffer (Cell Signaling, 9803), PMSF (Cell Signaling, 8553) and distilled water (dH₂O; BioConcept, 3-07F04-I), then sonicated and centrifuged. The supernatant was collected and used for immunoassay experiments, which were performed following the manufacturer’s instructions (Phoenix Peptide Somatostatin Fluorescent EIA Kit, EK-060-03).

Plasma hormone measurements

Insulin (Mercodia Ultrasensitive Mouse Insulin ELISA, 10-1249-01), GCG (Mercodia Glucagon ELISA, 10-1281-01), GLP-1 (Millipore Multi Species GLP-1 Total ELISA, EZGLP1T-36K), cortisol (R&D Systems Cortisol Parameter Assay Kit, KGE008B), growth hormone (Alpco Mouse/Rat Growth Hormone ELISA, 22-GHOMS-E01) and epinephrine (LSBio Mouse Adrenaline/Epinephrine ELISA Kit, LS-F28134) were measured in plasma samples obtained from blood extracts from the tail vein or cardiac puncture. A dipeptidyl peptidase 4 inhibitor (Merck, DPP4) was added to the blood samples to avoid GLP-1 degradation. All analyses were performed following the manufacturer’s instructions.

Hepatic glycogen assay

Approximately 30 mg of liver tissue was homogenized and boiled for 5 min. After centrifugation at 13,000g for 5 min at 4 °C, at least 50 μl of supernatant was collected for analysis. Glycogen was assessed using the Glycogen Assay Kit (Merck, MAK016-1KT).

Hepatic pyruvate and lactate assay

Approximately 30 mg of liver tissue was lysed in a solution of 10× Cell Lysis Buffer (Cell Signaling, 9803), PMSF (Cell Signaling, 8553) and dH₂O (BioConcept, 3-07F04-I), deproteinized in PCA (BioVision, K808-200) and neutralized (BioVision, K808-200) following the manufacturer’s instructions. Pyruvate (BioVision, K609-100) and lactate (BioVision, K607-100) were analysed following the manufacturer’s instructions.

Immunofluorescence

Paraffin and cryosections were 5 and 10 µm thick, respectively. The primary antibodies used were guinea pig anti-insulin (1:400; DAKO, A0564), rabbit anti-insulin (1:3,000; Molecular Probes, 701265), chicken anti-insulin (1:200; Abcam, ab14042); mouse anti-glucagon (1:1,000; Sigma-Aldrich, G2654), rabbit anti-glucagon (1:200; DAKO, A0565), mouse anti-somatostatin (1:200; BCBC, Ab1985), rabbit anti-somatostatin (1:200; DAKO, A0566), rat anti-somatostatin (1:200; Merck, Mab354) mouse anti-Ppy (1:400; Santa Cruz, MAB62971) and goat anti-Glp1 (1:100; Santa Cruz, sc-7782). Sections were also stained with DAPI. Secondary antibodies were coupled to Alexa 488, 405, 568, 647 (1:500; Molecular Probes) or TRITC (1:500; Southern Biotech). All antibodies are listed in Supplementary Table 3. All sections were examined with a confocal microscope (Leica TCS SPE).

Body composition

Body composition was determined in awake mice by magnetic resonance using EchoMRI-700 (EchoMRI). Body composition is expressed as a percentage of body weight (that is, percent of lean and fat mass).

Hyperinsulinemic–euglycaemic clamp

Hyperinsulinemic–euglycaemic clamps were performed in conscious, unrestrained, catheterized mice as previously described⁸⁴. In brief, catheters were surgically implanted 7 days before the experiment in the right jugular vein and exteriorized above the neck using a vascular access button (Instech Laboratories). Mice were fasted for 3 h, followed by a 2 h infusion of [3-³H] glucose (0.05 μCi min⁻¹) (Perkin Elmer). The basal rate of glucose disappearance (mg glucose kg⁻¹ of body weight × min⁻¹) was determined by blood sampling in duplicate. Continuous insulin infusion (2.5 mIU kg⁻¹ body weight × min⁻¹; Actrapid, Novo Nordisk) was used after that for the induction of hyperinsulinaemia. At steady state, hepatic glucose production (mg glucose kg⁻¹ of body weight × min⁻¹) and the insulin-stimulated rate of glucose disappearance (mg of glucose kg⁻¹ of body weight × min⁻¹) were determined by two blood samplings. The in vivo insulin-stimulated glucose uptake in tissues was then determined by a 10 μCi bolus intravenous injection of 2-[¹⁴C] deoxyglucose. After 30 min, mice were rapidly killed by cervical dislocation, and tissues were removed and stored at −80 °C until use. Measurements of 2-[¹⁴C] deoxyglucose-6-phosphate concentration in individual tissues allowed calculation of the glucose utilization index in tissues. Glycaemia was measured using an Xpress glucometer, and basal and steady-state insulinaemia were determined using a commercial ELISA kit (CrystalChem).

Glucose uptake

In vivo insulin-stimulated glucose uptake in tissues was determined by a 20 μCi bolus intravenous injection of 2-deoxy-[1,2-3H]-glucose (ARC) in the presence of insulin (NovoRapid) at 0.5 IU kg⁻¹ intraperitoneally. Blood was sampled from the tail vein 2, 20, 40 and 60 min after injections. After 1 h, mice were killed and tissues were collected and stored at −80 °C until use. Glucose concentration in deproteinized blood samples was measured using the glucose oxidase method (Roche Diagnostics). Measurements of [1,2-3H] deoxyglucose-6-phosphate levels in deproteinized blood samples and individual tissues allowed calculation of the glucose utilization index in tissues.

Islet isolation for perifusion assays

Islets were isolated from the pancreas of 7 h-fasted donor mice by collagenase digestion (0.45 mg ml⁻¹) and purified by a discontinuous Ficoll density gradient. After isolation, islets were hand-picked in RPMI-1640 medium supplemented with 5% (v/v) FCS (Gibco), 1% (v/v) l-glutamine (Gibco), 1% (v/v) penicillin–streptomycin (Sigma-Aldrich) and 5.5 mM glucose (Merck). Islets were allowed to rest free-floating for 18–24 h before islet perifusion assays at 37 °C and 5% CO₂.

Pancreas tissue slices

Pancreas tissue slices were performed on 7 h-fasted mice as described previously^22,85. In brief, pancreata were injected with 1.25% low-melting-point agarose (Roth) after killing the mouse. After solidification, the pancreas was excised and embedded in agarose (1.25%). Tissue blocks were subjected to a semiautomated vibratome (Leica) and pancreas tissue slices were cut in ECS solution (125 mM NaCl, 2.5 mM KCl, 26 mM NaHCO₃, 1.25 mM NaH₂PO₄, 1 mM MgCl₂, 2 mM CaCl₂, 10 mM HEPES, 3 mM glucose pH 7.4) at a thickness of 150 µm. Slices were collected into a 6 cm Petri dish containing 3 mM glucose KRBH buffer (137 mM NaCl, 5.36 mM KCl, 0.34 mM Na₂HPO₄, 0.81 mM MgSO₄, 4.17 mM NaHCO₃, 1.26 mM CaCl₂, 0.44 mM KH₂PO₄, 10 mM HEPES, 0.1% BSA, 3 mM glucose pH 7.3) with aprotinin (25 KIU ml⁻¹, Sigma-Aldrich, A6106) and allowed to rest for 120 min at room temperature (20–22°C) while shaking before performing slice perifusion experiments.

Perifusion assays and insulin secretion quantification

Dynamic insulin secretion of isolated islets and pancreas tissue slices was performed using a perifusion system with automated tray handling (Biorep Technologies, PERI4-02-230-FA). A total of 40 islets were placed into perifusion columns (Biorep Technologies, PERI-CHAMBER) according to the provided manual, whereby islets are placed between two layers of sedimented agarose beads. For pancreas tissue slice perifusion, three slices originating from different embedded blocks were placed into a closed perifusion chamber (Warner Instruments, 64-0223 and 64-0281 (P-5)) connected to the perifusion system. To equilibrate the islets or slices to 37 °C and to wash out accumulated hormones and enzymes, a 90-min flushing step with 3 mM glucose KRBH with aprotinin (25 KIU ml⁻¹, Sigma-Aldrich, A6106) at a flow rate of 100 µl min⁻¹ was performed. Subsequently, the perifusion protocols were applied using a flow rate of 100 µl min⁻¹ and sample collection in 96-well plates at 2-min intervals. Aprotinin (25 KIU ml⁻¹) was added to all KRBH buffers used for the different protocols. After perifusion, islets and slices were recovered from the columns and perifusion chambers and lysed for total insulin content measurement using 250 µl and 500 µl acid–ethanol (2% HCl (37 %, 12 M) in absolute ethanol), respectively. All samples were kept at −20 °C until measured with an Insulin Ultrasensitive HTRF Assay Kit (Perkin Elmer–Cisbio, 62IN2PEH).

In vitro static glucose-stimulated insulin secretion

Murine isolated islets or human pseudoislets were hand-picked for each assay replicate and washed by incubation for 1 h at 37 °C in secretion medium containing 2.5 mM CaCl₂, 140 mM NaCl, 4.5 mM KCl, 1 mM MgCl₂, 20 mM Hepes and 3 mM glucose (Sigma-Aldrich) in dH₂O. Samples were then transferred into fresh secretion medium containing 3 mM (low) glucose for 1 h, followed by incubation for another 1 h in secretion medium containing 16.7 mM (high) glucose at 37 °C. Then, 1 nM Ex-4 (Sigma-Aldrich, E7144) supplementation in the secretion medium containing 16.7 mM (high) glucose was added to assess the response of β-cells to the incretin agonist. The medium was collected after a 1 h incubation at each glucose concentration and stored at −80 °C for subsequent analysis. Islets and pseudoislets were recovered and lysed for total insulin content using acid–ethanol (74% ethanol, 1.4% HCl). Mouse insulin concentration was quantified using the Ultrasensitive Mouse Insulin ELISA (10-1249-01, Mercodia). Human insulin concentration was measured using the Insulin Chemiluminiscence ELISA (ALPCO, 80-INSHU-CH01).

XFe96 Seahorse islet respirometry

Mouse islets or human pseudoislets (8–10 per well) were seeded into wells of a poly-d-lysine-coated (100 mg ml⁻¹) XFe96 plate containing Seahorse XF base media RPMI (supplemented with 3 mM glucose, 10 mM HEPES, 2 mM glutamax, 30 mM NaCl and 0.1% FBS) as described previously⁸⁶. Before the assay, islets were incubated for 1 h at 37 °C in a non-CO₂ incubator. The Seahorse XFe96 extracellular flux analyser and the Mito Stress kit containing mitochondrial toxins (Agilent Technologies) were used to assess mitochondrial respiration and islet bioenergetics. Basal respiration was first measured at 3 mM glucose. Then, islets and pseudoislets were sequentially stimulated with glucose (final well concentration of 16.7 mM), oligomycin (2.5 μM), FCCP (2 μM) and a mixture of rotenone and antimycin A (Rot/AA, 3 μM). Islets and pseudoislets were recovered at the end of the assay and lysed for total insulin content using acid–ethanol (74% ethanol, 1.4% HCl).

OCR values were normalized by insulin content per well to reduce the confounding effect of non-β-cells in the measurements of the control samples. Then, a fold change to the basal respiration was calculated. Bioenergetics parameters were calculated as previously described⁸⁶. In brief, average values after injection of Rot/AA were subtracted from all OCR measurements. Glucose-stimulated OCR was calculated by dividing the maximum OCR measurement after 16.7 mM glucose injection by the last basal OCR measurement at 3 mM glucose. Proton leak was determined by dividing the minimum OCR value after oligomycin A stimulation by the last basal OCR value. Lastly, maximal respiration was calculated by dividing the maximal OCR value after FCCP injection by the last basal OCR value. All parameters were multiplied by 100 and are shown as % of basal.

HFD

Rodent diet with 60 kcal% fat (Research Diets, D12492) or diet with 10 kcal% fat (Research Diets, D12450J) were administered to control and β-only mice 1 month post ablation, for 24 weeks. The diet was changed every 2 days.

Metabolic cage (Labmaster)

Body mass composition was analysed before and after indirect calorimetric experiment using an EchoMRI-700 (EchoMRI). Mice were analysed for whole energy expenditure, oxygen consumption and carbon dioxide production, respiratory exchange rate (VCO₂/VO₂), food intake and spontaneous locomotor activity using calorimetric cages (Labmaster, TSE Systems). Activity was recorded using an infrared light beam-based locomotion monitoring system (beam breaks per 15 min). Spontaneous exercise activity was also recorded using running wheels (Columbus) inside the metabolic cage. Mice were individually housed and acclimated for 4 days before experimental measurements. Data analysis was carried out with Excel using extracted raw values of the last 5 days of VO₂ consumption, VCO₂ production (ml h⁻¹) and energy expenditure (kcal h⁻¹). Subsequently, each value was normalized per lean tissue mass extracted from the EchoMRI analysis.

Statistics and reproducibility

Statistical analyses were performed using Prism v.9.0 software, applying Mann–Whitney two-sided tests or one-way ANOVA for comparison (nonsignificant, P > 0.05; *P ≤ 0.05; **P ≤ 0.01; ***P ≤ 0.001; ****P ≤ 0.0001). P values are described in the figure legends and Source data tables. Significant statistical differences are indicated in the figures. More than three mice per condition and experiment were analysed as indicated in the figure legends and Source data tables. Immunofluorescence was performed more than once for each mouse with more than four paraffin or cryosections per mouse. The RNA sequencing experiment was performed once. pPCRs were performed using four to ten individual biological samples as indicated in figure legends; each biological sample was run in triplicate.

Reporting summary

Further information on research design is available in the Nature Portfolio Reporting Summary linked to this article.

Data availability

The mouse β-cell bulk RNA sequences generated in this study have been deposited in the NCBI GEO database (accession number GSE226479). All sequencing data were uploaded to and aligned on the Galaxy project80 against Ensembl reference genome GRCm38.p6 (release 100) (https://www.ensembl.org/Mus_musculus/Info/Index). The β-ID gene list generated in a previous publication⁷⁹ (NCBI GEO database, accession number GSE150724) was used for analysis. The unfiltered list of differentially expressed genes is provided as Supplementary Data. Source data for Figs. 1–6 and Extended Data figures are provided with this paper in the Source data files; the availability of associated source data is indicated in each figure legend. Donor details for human samples are available in Supplementary Table 4. All data and materials used are available from commercial sources as presented in the Methods and from the corresponding author on reasonable request. Source data are provided with this paper.

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Acknowledgements

We thank G. Gallardo, C. Gysler and B. Polat for technical help, S. Chera for the scientific discussions, J.-P. Aubry-Lachainaye and G. Schneiter for FACS assistance, M. Docquier for RNA sequencing advice and C. Veyrat-Durebex and F. Bontems for physiological and metabolic advice and support. Human pancreatic islets isolated from deceased (brain-dead) multiorgan donors were obtained from three different centres: (1) the NIDDK-funded integrated Islet Distribution Program (IIDP) at City of Hope (RRID: SCR_014387), National Institutes of Health grant no. 2UC4DK098085; (2) the Alberta Diabetes Institute IsletCore at the University of Alberta in Edmonton (http://www.bcell.org/adi-isletcore.html) with the assistance of the Human Organ Procurement and Exchange (HOPE) program, Trillium Gift of Life Network (TGLN) and other Canadian organ procurement organizations (islet isolation was approved by the Human Research Ethics Board at the University of Alberta (Pro00013094)); and (3) the Geneva University Hospital (CCER protocol 2016-01979; Laboratoire d’Isolement et de Transplantation Cellulaires, Dépt. de Chirugie), with approved islet use according to CCER protocol 2019-00518. This work was funded with grants from the Swiss National Science Foundation (nos. 310030_192496, 310030E_205640 and 320030_227816), the European Research Council (no. 884449; ‘Merlin’ Advanced Grant) and the Fondation Aclon to P.L.H., and the JST FOREST Program (#JPMJFR210Y) to K.F. The funders had no role in study design, data collection and analysis, decision to publish or preparation of the manuscript.

Author information

Kenichiro Furuyama
Present address: Center for iPS Cell Research and Application (CiRA), Kyoto University, Kyoto, Japan
These authors contributed equally: Fabrizio Thorel, Pedro L. Herrera.

Authors and Affiliations

Department of Genetic Medicine and Development, iGE3 and Centre facultaire du diabète, Faculty of Medicine, University of Geneva, Geneva, Switzerland
Marta Perez-Frances, Eva Bru-Tari, Maria Valentina Abate, Léon van Gurp, Kenichiro Furuyama, Fabrizio Thorel & Pedro L. Herrera
Institute of Physiology, Faculty of Medicine, Technische Universität Dresden, Dresden, Germany
Christian Cohrs & Stephan Speier
Paul Langerhans Institute Dresden of the Helmholtz Zentrum München at the University Clinic Carl Gustav Carus of Technische Universität Dresden, Helmholtz Zentrum München, Neuherberg, Germany
Christian Cohrs & Stephan Speier

Authors

Marta Perez-Frances
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Eva Bru-Tari
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Christian Cohrs
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Maria Valentina Abate
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Léon van Gurp
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Kenichiro Furuyama
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Stephan Speier
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Fabrizio Thorel
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Pedro L. Herrera
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Contributions

M.P.F. conceived and performed the experiments and analyses and wrote the paper. E.B.T. conceived and performed the human islet experiments and analysis and wrote the paper. C.C. and S.S. performed the dynamic insulin secretion experiments. M.V.A. developed and bred the non-β-DTR mouse line. L.v.G. analysed the transcriptomic data. K.F. conceived the human islet experiments. F.T. and P.L.H. generated the non-β-DTR mouse line, conceived the experiments, interpreted the observations and wrote the paper.

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Correspondence to Pedro L. Herrera.

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Nature Metabolism thanks Gordon Weir and the other, anonymous, reviewer(s) for their contribution to the peer review of this work. Primary Handling Editors: Revati Dewal and Isabella Samuelson, in collaboration with the Nature Metabolism team.

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Extended data

Extended Data Fig. 1 Long-term characterization of aged mice 40-weeks after non-β-cell ablation.

a. Immunofluorescence on pancreas tissue sections from control (Ctrl) or DT-treated mice analyzed 40 weeks post-ablation (wpa). INS: red; GCG: green (left); INS: red; SST: green (middle); INS: red; PPY: green (right). Scale bar: 20 µm. b. Quantification of GCG+, SST+, and PPY+ cells in Ctrl (black) or DT (red) mice 40wpa. GCG+ and SST+ (Ctrl n = 7, DT n = 5) cells were scored in the dorsal region of the pancreas; PPY+ (Ctrl n = 3, DT n = 5) cells were scored in the ventral region of the pancreas. P-values Ctrl vs DT: GCG + P = 0.0025, SST + P = 0.0025, PPY + P = 0.036. c. Pancreatic insulin content (ng/mg) of Ctrl (black, n = 6) and DT (red, n = 6) mice 40wpa. P-value Ctrl vs DT = 0.937. Only male mice were used. All data are shown as mean ± sem. All statistical tests are two-tailed Mann-Whitney test. Source data is available.

Source data

Extended Data Fig. 2 Somatostatin-producing intestinal D-cell ablation and regeneration in β-only mice.

a, Body weight over 40weeks on Ctrl (black, n = 6) and DT (red, n = 6) mice in random fed (RF, continuous line) and fasting (F, dashed line). Right panel: Area under the curve (AUC). P-values (DTvsCtrl): RF P = 0.3312, F P = 0.3939. b, Body composition in Ctrl (black, n = 8) and DT (red, n = 8) mice. P-values CtrlvsDT: Lean mass P = 0.7209, Fat mass P = 0.083. c, Immunofluorescence on SST (red) in stomach (upper micrographs) and GLP-1 (red) in colon (lower micrographs) from Ctrl or β-only mice. Scale bar: 20 µm or 10 µm (insets). d, Duodenum qPCR of Sst of Ctrl (black, n = 4) and β-only mice at 7 dpa (pink, n = 7), 15 dpa (light red, n = 7), and 30 dpa (red, n = 6). Data are normalized ct values relative to β-actin and Gapdh and shown as relative hormone expression to Ctrl. P-values: 7 dpa vs Ctrl P = 0.0061, 15 dpa vs Ctrl P = 0.0606, 30 dpa vs Ctrl P = > 0.999. e, Plasma somatostatin in Ctrl (n = 16) and β-only after 15 dpa (pink, n = 8) and 30 dpa (red, n = 8). P-values: 15 dpa vs Ctrl P = 0.0016, 30 dpa vs Ctrl P = 0.1090, 30 dpa vs 15 dpa P = 0.0468. f, Brain qPCR on Sst of Ctrl (black, n = 4) and β-only (red, n = 6). Data are normalized ct values relative to β-actin and Gapdh and shown as relative hormone expression to Ctrl. P-values Ctrl vs DT: P = 0.0095. g, Brain somatostatin of Ctrl (n = 8) and β-only (n = 7). P-values: DT vs Ctrl P = 0.0128. h-j, Food intake (h; gr/gr), total movement (i; counts, infrared breaks in 15 minutes) and running wheel activity (j) in Ctrl (black, n = 9) and DT (red, n = 7). Right panel: AUC. Food intake (h) P-value (CtrlvsDT): light period P = 0.2523; dark period P = 0.6065; 24 h P = 0.4079. Total movement (i) P-value (CtrlvsDT): light period P = 0.2105; dark period P = 0.8371; 24 h period P = 0.7577. Running wheel (j) P-value (CtrlvsDT): light period P = > 0.99; dark period P = 0.9182; 24 h period P = > 0.99. Only male mice were used. All data are shown as mean ± sem. All statistical tests are two-tailed Mann-Whitney test. Source data is available.

Source data

Extended Data Fig. 3 Improved blood glucose homeostasis in female β-only mice.

a. Glycemia over 40 weeks post-ablation of Ctrl (black; n = 9) and DT (red; n = 10) female mice in random-fed (RF, continuous line) or fasting (F, dashed line). Right panel: area under the curve (AUC) of glycemia. P-values (DT vs Ctrl): RF P = 0.0038; F P = 0.067. b. Body weight over 40 weeks post-ablation of Ctrl (black; n = 9) and DT (red; n = 10) female mice in RF (continuous line) or F (dashed line). Right panel: AUC of body weight. P-values DT vs Ctrl: RF P = 0.468; F P = 0.2013. c. Intraperitoneal glucose tolerance test (ipGTT) at 4wpa. Left panel: ipGTT on Ctrl (black; n = 17) and DT (red; n = 18). Right panel: AUC of ipGTT; P-value (Ctrl vs DT) P = 0.3142. d. Plasma insulin along ipGTT. Left panel: plasma insulin at 0 and 15 minutes after glucose injection in Ctrl (black; n = 12) and DT (red; n = 7) mice. Right panel: stimulation index (S.I.) of insulin secretion. P-value (Ctrl vs DT) P = 0.0646. e. Oral glucose tolerance test (oGTT) at 30 dpa. Left panel: oGTT on Ctrl (black; n = 10) and DT (red; n = 7). Right panel: AUC of oGTT. P-value (Ctrl vs DT) = 0.0431. f. Plasma insulin along oGTT. Left panel: plasma insulin at 0 and 10 minutes after glucose gavage in Ctrl (black; n = 10) and DT (red; n = 6) mice. Right panel: stimulation index (S.I.) of insulin secretion. P-value Ctrl vs DT P = 0.2424. g. Insulin tolerance test (ITT) at 30 dpa. Left panel: ITT on Ctrl (black; n = 8) and DT (red; n = 7) mice. Data are shown as % relative to glycemia at time 0. Right panel: AUC of ITT. P-value Ctrl vs DT P = 0.0093. Error bars denote s.e.m. Two-tailed Mann-Whitney test. Source data is available.

Source data

Extended Data Fig. 4 Blood glucose homeostasis in mice without somatostatin-expressing δ-cells.

a, Pancreas immunofluorescence from control (Ctrl) or δ-cell ablated mice. INS: red; SST: green. Scale bars: 20 µm. b. Quantification of SST+ cells per islet section in Ctrl (black, n = 3) or DT (red, n = 3) mice (dorsal pancreas). P-values CtrlvsDT P = 0.0007. c, Plasma somatostatin (ng/ml) in Ctrl (black, n = 11) and DT (red, n = 8). P-values CtrlvsDT: P = 0.0157. d, Glycemia of Ctrl (black, n = 6) and DT (red, n = 6) in RF (continuous line) or F (dashed line). Right panel: area under the curve (AUC). P-values: RF DTvsCtrl P = 0.0043; F DTvsCtrl P = 0.8182. e, Body weight change (% from day 0) of Ctrl (black, n = 6) and DT (red, n = 6) in random-fed. Right panel: AUC. P-values: RF DTvsCtrl P = 0.0043. f, Intraperitoneal glucose tolerance test (ipGTT) on Ctrl (black, n = 9) and DT (red, n = 10). Right panel: AUC; P-value CtrlvsDT P = 0.0279. g, Plasma insulin at 0 and 15 minutes after glucose in Ctrl (black, n = 8) and DT (red, n = 10). P-value Ctrl (0’ vs 15’) = 0.0140; DT (0’ vs 15’) = 0.0015. h, Insulin tolerance test (ITT) on Ctrl (black, n = 9) and DT (red, n = 10). Data are shown as % relative to glycemia at time 0. Right panel: AUC; P-value CtrlvsDT=0.0789. i, Oral glucose tolerance test (oGTT) on Ctrl (black, n = 8) and DT (red, n = 10). Right panel: AUC; P-value (CtrlvsDT) = 0.0055. j, Plasma insulin at 0 and 10 minutes after glucose in Ctrl (black, n = 7) and DT (red, n = 10). P-value Ctrl (0’ vs 10’) = 0.0041; DT (0’ vs 10’) = 0.0011. Right panel: stimulation index (S.I.) of insulin; P-value (CtrlvsDT)=0.9623. k, Plasma GLP-1 along oGTT in Ctrl (black, n = 9) and DT (red, n = 9). P-value (CtrlvsDT)=0.0056. Only male mice were used. Data are shown as mean ± sem. Statistical tests are two-tailed Mann-Whitney. Source data is available.

Source data

Extended Data Fig. 5 Hyperinsulinemic-euglycemic clamp after non β-cell ablation.

a, Experimental time-line for the hyperinsulinemic-euglycemic clamp. 2.5mUI/kg/min of insulin were continuously infused during the insulin clamp. Blood samples were taken at multiple time for further analyses. b-c, Glucose infusion rate (GIR, b) and hepatic glucose production (HGP, c) measured during clamp studies in Ctrl (black, n = 7) and DT (red, n = 6) mice. P-values: CtrlvsDT HGP P = 0.007. d-f, Radiolabeled 2-deoxy-D-glucose (2DG) uptake by adipose tissue in Ctrl (black, n = 7) and DT (red, n = 6) mice. P-values (Ctrl vs DT): Brown Adipose Tissue (BAT) P = 0.073; subcutaneous White Adipose Tissue (sWAT) P = 0.008; inguinal White Adipose Tissue (iWAT) P = 0.005. Insulin clamp and 2DG uptake were obtained from the same mice. Only male mice were used. All data are shown as mean ± sem. All statistical tests are two-tailed Mann-Whitney test. Source data is available.

Source data

Extended Data Fig. 6 High-fat diet administration to β-only mice.

a, Food intake (gr) of Ctrl+Chow (grey, n = 6), Ctrl+HFD (black, n = 5), DT+Chow (pink, n = 4), DT + HFD (red, n = 6) over the last 4-weeks of high-fat diet (HFD). Right panel: area under the curve (AUC). P-values: Ctrl+chow vs Ctrl+HFD P = 0.7922, Ctrl+chow vs DT+chow P = 0.4762, Ctrl+chow vs DT + HFD P = 0.0649, Ctrl+HFD vs DT+chow P = 0.9048, Ctrl+HFD vs DT + HFD P = 0.6623; DT+chow vs DT + HFD P = 0.4762. b, Random fed glycemia of Ctrl+Chow (grey, n = 10), Ctrl+HFD (black, n = 10), DT+Chow (pink, n = 8), DT + HFD (red, n = 11) over 24 weeks of HFD. Right panel: AUC. P-values: Ctrl+chow vs Ctrl+HFD P < 0.62, Ctrl+chow vs DT+chow P = 0.12, Ctrl+chow vs DT + HFD P = 0.13, Ctrl+HFD vs DT+chow P = 0.03, Ctrl+HFD vs DT + HFD P = 0.04; DT+chow vs DT + HFD P = 0.97. c, Intraperitoneal glucose tolerance test (ipGTT) 24-weeks after HFD of Ctrl+chow (grey, n = 10), Ctrl+HFD (black, n = 10), DT+chow (pink, n = 8), DT + HFD (red, n = 11). Right panel: AUC. P-values: Ctrl+chow vs Ctrl+HFD P = 0.0073, Ctrl+chow vs DT+chow P = 0.0.0038, Ctrl+chow vs DT + HFD P = 0.9404, Ctrl+HFD vs DT+chow P < 0.0001, Ctrl+HFD vs DT + HFD P = 0.0012; DT+chow vs DT + HFD P = 0.0129. d, Plasma insulin release at 0 and 15 minutes after glucose injection in Ctrl+chow (grey, n = 9), Ctrl+HFD (black, n = 10), DT+chow (pink, n = 8), DT + HFD (red, n = 11). P-values: Ctrl+Chow (0’vs15’) P = 0.0039; Ctrl+HFD (0’vs15’) P = 0.0355; DT+Chow (0’vs15’) P = 0.0281; DT + HFD (0’vs15’) P = 0.0192. Ctrl+HFD vs DT + HFD at 0’ P = 0.0357; Ctrl+HFD vs DT+Chow at 15’ P = 0.0044; Ctrl+HFD vs DT + HFD at 15’ P = 0.0101. Only male mice were used. All data are shown as mean ± sem. All statistical tests are two-tailed Mann-Whitney test. Source data is available.

Source data

Extended Data Fig. 7 Improved glucose homeostasis after the specific ablation of the pancreatic α-, δ-, and γ-cells.

a. Immunofluorescence from control (Ctrl, left panel), mice injected with 120 ng of DT (middle panel) or 5 ng of DT (right panel). Top row: Brain somatostatin (green). Mid row: islet insulin (red), glucagon, somatostatin or Ppy (green). Bottom row: stomach somatostatin (green). Scale bars: 20 μm or 10 μm (insets). b. Brain qPCR on SST in Ctrl (black; n = 6) and 120ngDT (grey; n = 3) or 5ngDT (red; n = 5). Data are normalized ct values relative to β-actin and Gapdh. P-values: Ctrlvs5ngDT P = 0.6623, Ctrlvs120ngDT P = 0.0238, 5ngDTvs120ngDT P = 0.0357. c. Quantification of pancreatic GCG+, SST+, and PPY+ cells in Ctrl (black; n = 5), 120ngDT (grey; n = 4) or 5ngDT (red; n = 4). P-values: GCG+ Ctrlvs5ngDT P < 0.0001, Ctrlvs120ngDT P < 0.0001, 5ngDTvs120ngDT P = 0.5783. SST+ Ctrlvs5ngDT P = 0.0001, Ctrlvs120ngDT P < 0.0001, 5ngDTvs120ngDT P = 0.9852. PPY+ Ctrlvs5ngDT P < 0.0001, Ctrlvs120ngDT P < 0.0001, 5ngDTvs120ngDT P = 0.9964. d. Stomach qPCR on SST in Ctrl (black; n = 14) and 120ngDT (grey; n = 4) or 5ngDT (red; n = 4). Data are normalized ct values relative to β-actin and Gapdh. P-values: Ctrlvs5ngDT at 15 dpa P = 0.0013; Ctrlvs5ngDT at 30 dpa P = 0.7209; Ctrlvs120ngDT at 15 dpa P = 0.0006; Ctrlvs120ngDT at 30 dpa P = 0.0676; 5ngDT 15dpavs30dpa P = 0.0286; 120ngDT 15dpavs30dpa P = 0.0043. e-f. Glycemia (e) and body weight (f, % of change) of Ctrl (black; n = 12), 120ngDT (grey; n = 7) or 5ngDT (red; n = 8). Small panel: area under the curve (AUC). P-values: Glycemia Ctrlvs5ngDT P = 0.0017; Ctrlvs120ngDT P < 0.0001; 5ngDTvs120ngDT P = 0.003. Body weight Ctrlvs5ngDT P = 0.1196; Ctrlvs120ngDT P < 0.0001; 5ngDTvs120ngDT P = 0.003. g. Oral glucose tolerance test (oGTT) in Ctrl (black; n = 14), 120ngDT (grey; n = 10) or 5ngDT (red; n = 8). P-values: Ctrlvs5ngDT P = 0.0003; Ctrlvs120ngDT P < 0.0001; 5ngDTvs120ngDT P = 0.4215. h. Stimulation index (S.I.) of insulin in Ctrl (black; n = 12), 120ngDT (grey; n = 10) or 5ngDT (red; n = 8). P-values Ctrlvs5ngDT P = 0.0011; Ctrlvs120ngDT P = 0.0206; 5ngDTvs120ngDT P = 0.2844. i. Insulin tolerance test (ITT) in Ctrl (black; n = 14), 120ngDT (grey; n = 9) or 5ngDT (red; n = 8). Data are shown as % relative to glycemia at time 0. Right panel: AUC. P-values Ctrlvs5ngDT P = 0.0072; Ctrlvs120ngDT P = 0.0005; 5ngDTvs120ngDT P = 0.7979. j. Graphical summary. Only male mice were used. Error bars denote s.e.m. Two-way ANOVA and two-tailed Mann-Whitney test are used. Source data is available.

Source data

Extended Data Fig. 8 Ex vivo dynamic insulin secretion in pancreatic slices and isolated islets.

a, Pancreatic insulin content (ng) of slices from control (Ctrl, black, n = 5) and DT (red, n = 3). P-value CtrlvsDT=0.250. b, Area under the curve (AUC) of the first phase (grey area, 14- and 24-minutes) and second phase (dashed grey area, 30- and 58-minutes). P-values (CtrlvsDT): first phase P = 0.393; second phase P = > 0.999. c-d, Islet equivalent count (IEQ, c) and ratio insulin content (ng) and IEQ count (d) of Ctrl (black, n = 9) and DT (red, n = 8). P-value: IEQ count (CtrlvsDT) P = 0.2359; ratio insulin content and IEQ (CtrlvsDT) P = 0.743. e, AUC of first phase (P-value CtrlvsDT P = 0.393) and second phase (P-value CtrlvsDT P = > 0.999) of insulin secretion in isolated islets of Ctrl (black; n = 9) and DT (red; n = 8) mice. f, Total insulin content (ng) of isolated islets from Ctrl (black, n = 7) and DT (red, n = 10) mice with or without Exendin-4 (Ex-4). P-value without Ex-4 CtrlvsDT P = 0.601; P-value with Ex-4 CtrlvsDT P = 0.3031. g-h. Islet respirometry parameters. g. Glucose-stimulated OCR (dashed lined column), proton leak and maximal respiration (grey column) in islets from Ctrl (black, n = 8) and DT (red, n = 7) mice. P-values (CtrlvsDT): Glucose-stimulated OCR P = 0.3285; Proton leak P = 0.2046; Maximal respiration P = 0.999. h. Basal respiration measured at 3 mM glucose from Ctrl (black, n = 8) and DT (red, n = 7). 2-4 wells/mice, 8-10 islets/well. P-values Ctrl vs DT P = 0.281. i. Total insulin content of islets from Ctrl (black, n = 8) and DT (red, n = 7) after OCR measurements. P-values CtrlvsDT P = 0.3357. Each data point (g-i) represents the average values per mouse. Only male mice were used. All data are shown as mean ± sem. All statistical tests are two-tailed Mann-Whitney test. Source data is available.

Source data

Extended Data Fig. 9 Transcriptomic analysis of β-cells isolated from control and β-only mice.

a, Experimental design. b, Representative gating strategy used for FACS sorting the mCherry+ insulin-expressing cells in Ctrl and β-only mice for RNA-seq analysis. c, Principal component analysis (PCA) of RNA-seq samples. Each dot represents one sample. Four different conditions: Control Fasting (Ctrl F, green, n = 5), DT Fasting (DT F, red, n = 6), Control Refed (Ctrl RF, blue, n = 5) and DT Refed (DT RF, yellow, n = 6). d-e, MA plot of the DEGs (differentially expressed genes) between DT and Ctrl during 8-hour fasting (d) and after 2-hour refeeding (e). Each dot represents one gene. Red dots are the genes with p-values < 0.05 and a log fold change >0.5 or <−0.5. f, Heatmap showing scaled expression (blue, high expression; white, low expression) of representative β-ID genes. The dendrogram represents the clustering of each condition analyzed based on β-ID genes expression. g, Expression levels of key identity (top panel) and functional (bottom panel) β-cell genes during fasting in controls and DT-treated mice after 8-hour fasting or 2-refeeding. P-values for all genes and conditions are non significant (P > 0.05). Only male mice were used. Data are shown as mean ± sd. All statistical tests are two-tailed Mann-Whitney test. Source data is available.

Source data

Extended Data Fig. 10 Stimulatory index and glucose-stimulated oxygen consumption are maintained in human monotypic β-pseudoislets.

a. FACS strategy used to purify human β-cells. Representative plots of cells labelled with the pan-endocrine marker HIC1-2B4, the non-β-cell endocrine marker H1C3-2D12 and the δ-cell enriched marker CD9. b. Stimulation index of absolute insulin secretion at 16.7 mM glucose in presence/absence of the GLP-1 agonist Exendin-4 (Ex-4, 50 nM) in pseudoislets composed by all cell types (Ctrl, black) and only β-cells (red). Values are expressed as fold change to baseline values measured at 3 mM glucose (low glucose, LG). N = 4 donors. c. Total insulin content of control (black) and β-only pseudoislets (red) measured after stimulation at 16.7 mM glucose (high glucose, HG). N = 4 donors. P-values (Ctrl vs β): HG P = 0.9708, HG+Ex4 P = 0.4343. P-values Ctrl HG vs HG+Ex4 P = 0.8848. P-values β HG vs HG+Ex4 P = 0.9843. d-f. Pseudoislet respirometry parameters from Fig. 6e. N = 3 independent donors. 2-5 wells/condition/donor, 10 pseudoislets/well. Each data point represents the well average per donor. d. Glucose-stimulated OCR (dashed lined column), proton leak and maximal respiration (grey column) in control (black) and monotypic β-pseudoislets. P-values (Ctrl vs β): Glucose-stimulated OCR P = 0.872; Proton leak P = 0.539; Maximal respiration P = 0.982. (red). e. Basal respiration measured at 3 mM glucose before injections. P-values Ctrl vs β P = 0.4. f. Total insulin content of control (Ctrl) and β-pseudoislets (red) after OCR measurements. P-values Ctrl vs β P = 0.7. Both male and female human donors were used. All data are shown as mean ± sem. All statistical tests are two-tailed Mann-Whitney test. Source data is available.

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Supplementary information

Reporting Summary

Supplementary Tables 1–4

Supplementary Table 1: Summary of the phenotype after single or combined cell ablation. Supplementary Table 2: List of qPCR primers. Supplementary Table 3: List of antibodies used for immunofluorescence. Supplementary Table 4: Human donor information.

Supplementary Data 1 and 2

Supplementary Data 1: Differentially expressed genes between β-cells in control and β-only upon 8-h fasting. Supplementary Data 2: Differentially expressed genes in β-cells in control and β-only upon 8-h fasting followed by 2-h refeed.

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Perez-Frances, M., Bru-Tari, E., Cohrs, C. et al. Regulated and adaptive in vivo insulin secretion from islets only containing β-cells. Nat Metab (2024). https://doi.org/10.1038/s42255-024-01114-8

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Received: 26 April 2023
Accepted: 22 July 2024
Published: 21 August 2024
DOI: https://doi.org/10.1038/s42255-024-01114-8
Springer Nature Limited

Regulated and adaptive in vivo insulin secretion from islets only containing β-cells

Abstract

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Main

Results

Generation of a mouse model of islet non-β-cell loss

Proper glucose homeostasis in β-only mice

Improved glucose homeostasis in β-only mice on a high-fat diet

Islet non-β-cell loss drives the phenotype of β-only mice

β-only islets have a normal insulin secretion profile

Human β-cell pseudoislets display optimal insulin secretion

Discussion

Methods

Animals

DT and S961 treatment

Human islets and generation of human pseudoislets

Islet isolation, FACS and RNA extraction

RT–qPCR

Bulk RNA sequencing

Glucose tolerance test

Insulin tolerance test

Tissue protein extracts

Plasma hormone measurements

Hepatic glycogen assay

Hepatic pyruvate and lactate assay

Immunofluorescence

Body composition

Hyperinsulinemic–euglycaemic clamp

Glucose uptake

Islet isolation for perifusion assays

Pancreas tissue slices

Perifusion assays and insulin secretion quantification

In vitro static glucose-stimulated insulin secretion

XFe96 Seahorse islet respirometry

HFD

Metabolic cage (Labmaster)

Statistics and reproducibility

Reporting summary

Data availability

References

Acknowledgements

Author information

Authors and Affiliations

Contributions

Corresponding author

Ethics declarations

Competing interests

Peer review

Peer review information

Additional information

Extended data

Supplementary information

Source data

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