β-Cell Dysfunction Due to Increased ER Stress in a Stem Cell Model of Wolfram Syndrome

All forms of diabetes are ultimately the result of an inability of pancreatic β-cells to provide sufficient insulin in response to ambient blood glucose concentrations. Stem cell–based models of diabetes should enable analysis of specific pathways leading to human β-cell failure and the testing of strategies to preserve or restore β-cell function.

Childhood-onset insulin-dependent diabetes can be caused by mutations in WFS1 gene (wolframin), which is highly expressed in human islets as well as in the heart, brain, placenta, and lung (1). Wolfram syndrome subjects are also affected by optic atrophy, deafness, ataxia, dementia, and psychiatric illnesses (2). The disease is fatal, and no treatments for the diabetes other than provision of exogenous insulin are available. Postmortem analyses of pancreata of Wolfram patients show a selective loss of pancreatic β-cells (3). In the mouse, loss of the WFS1 gene results in impaired glucose-stimulated insulin secretion and a reduction of β-cells in pancreatic islets (4,5). But unlike human subjects, these mice develop only mild or no diabetes (4). Several molecular mechanisms by which WFS1 deficiency might affect β-cell function have been described. WFS1 deficiency reduces insulin processing and acidification in insulin granules of mouse β-cells, where low pH is necessary for optimal insulin processing and granule exocytosis (6). In human fibroblasts, WFS1 localizes to the endoplasmic reticulum (ER) (7), where it increases free Ca²⁺ (8) and interacts with calmodulin in a Ca²⁺-dependent manner (9). In mouse islets, following stimulation with glucose, WFS1 is found on the plasma membrane, where it appears to stimulate cAMP synthesis through an interaction with adenylyl cyclase, thereby promoting insulin secretion (10). In addition, WFS1 deficiency is accompanied by activation of components of the unfolded protein response (UPR), such as GRP78 (78 kDa glucose-regulated protein)/Bip (Ig-binding protein) and XBP-1 (X-box-binding protein-1) and reduced ubiquitination of ATF6α (activating transcription factor-6α) (11,12). Because the relevance of these molecular mechanisms to β-cell dysfunction is unclear, and because of phenotypic differences between mice and human subjects, there is a need for a biological model of the consequences of WFS1 deficiency in the human β-cells.

We generated insulin-producing cells from skin fibroblasts of patients with Wolfram syndrome and found that these WFS1 mutant cells display insulin processing and secretion in response to various secretagogues comparable to healthy controls but have a lower insulin content and increased activity of UPR pathways. The chemical chaperone, 4-phenyl butyric acid (4PBA), reduced the activity of UPR pathways and restored insulin content to levels comparable to controls. Experimental ER stress induced by exposure to low concentrations of thapsigargin (TG), impaired insulin processing, and abolished insulin secretion in response to various secretagogues, while β-cell function in control cells was unaffected. Importantly, genetic rescue of WFS1 restored insulin content and preserved the ability to secrete insulin under conditions of ER stress. These results demonstrate that ER stress plays a central role in β-cell dysfunction in Wolfram syndrome and identify a potential approach to clinical intervention.

Skin biopsies were obtained from subjects WS-1 (biopsy 1–088) and WS-2 (biopsy 1–071) at the Naomi Berrie Diabetes Center using a 3 mm AcuPunch biopsy kit (Acuderm Inc.). Skin fibroblasts were derived and grown as previously described. Fibroblast cells from WS-3, WS-4, and WFS1 mutation carrier were obtained from Coriell Research Institute. Induced pluripotent stem (iPS) cells were generated using the CytoTune-iPS Sendai Reprogramming Kit (Invitrogen) (13) or using retroviral vectors (14). To genetically rescue the WFS1 locus, Wolfram iPS cell lines were transfected with lentivirus containing wild-type WFS1 cDNA sequence (from Addgene plasmid 13011) under murine stem cell virus promoter. Cell lines with stable integration were selected and maintained by puromycin treatment.

Human embryonic stem (ES) or iPS cells were dissociated by dispase (3–5 min) and Accutase (5 min; Sigma). Cells were suspended in human ES medium containing 10 μmol/L Y27632, a rho-associated protein kinase inhibitor, and filtered through a 70 μm cell strainer. Then cells were seeded at a density of 800,000 cells/well in 12-well plates. After 1 or 2 days, when cells reached 80–90% confluence, differentiation was performed as previously described (15). To quantify the number of insulin-positive cells within β-cell cultures, and to simultaneously quantify insulin and proinsulin content within β-cells, cells were dissociated to single cells and divided into three fractions: 20% of cells for quantification of positively stained cells using a Celigo Cytometer system (Cyntellect), 40% for RNA analysis, and 40% for ELISA assay to determine insulin content. For insulin content analysis, cells were lysed by M-PER protein extraction reagent (Thermo Scientific). Proinsulin and insulin content was measured with human proinsulin and insulin ELISA kits (Mercodia). To determine insulin and glucagon secretion in live cultures, β-cells were washed for 1 h in CMRL medium then incubated in CMRL medium containing 5.6 mmol/L glucose for 1 h, and the medium was collected. After that, CMRL medium containing 16.9 mmol/L glucose, 15 mmol/L arginine, 30 mmol/L potassium, 1 μmol/L Bay K8644, or 1 mmol/L dibutyl cAMP (DBcAMP) + 16.9 mmol/L glucose was added to the wells for 1 h, and the medium was collected. Human C-peptide concentration was measured by ultrasensitive human C-peptide ELISA kit (Mercodia), which specifically detects C-peptide, but not insulin or proinsulin. Glucagon levels in medium were measured with a glucagon ELISA kit (ALPCO Diagnostics).

iPS cells, fibroblasts, or β-cells were incubated for the indicated time and concentration of TG, tunicamycin (TM; Sigma), sodium 4PBA, or tauroursodeoxycholate (TUDCA; both from EMD Chemicals Inc.) was added 1 h prior to and during TG or TM treatment. For long-term 4PBA treatment, cells were incubated with 1 mmol/L 4PBA from day 9 to day 15 of differentiation. Primers for PCR analysis of XBP-1 gel-imaging (16), sXBP-1 for quantitative PCR (17), ATF4 (18), GRP78, and insulin are listed in Supplementary Table 1.

RNA was isolated using RNAeasy plus kit (Qiagen). cDNA was generated by using a reverse transcriptase kit (Promega). Cells were lysed by using M-PER mammalian protein extraction reagent and NE-PER Nuclear and Cytoplasmic Extraction Kit (Thermo Scientific). Protein levels were determined by Western blot using the antibodies as listed: rabbit anti-ATF6α (ab37149, Abcam), rabbit anti-phospho-eIF2α (3597; Cell Signaling Technology), mouse anti-eIF2α (2103; Cell Signaling Technology), and mouse-anti-GRP78 antibody (sc-166490; Santa Cruz Biotechnology).

For electron microscopic analysis, differentiated β-cells were fixed in 2.5% glutaraldehyde in 0.1 mol/L Sorenson’s buffer (pH 7.2) for 1 h. Samples were processed and imaged by the Diagnostic Service, Department of Pathology and Cell Biology, Columbia University. Secretory granule structure and ER morphology were visually recognized. The number of granules per cell was determined using ImageJ software.

At 12 days of differentiation, 2–3 million cells were detached using TrypLE (Invitrogen), pelleted, and mixed with 10–15 μl matrigel (BD Biosciences) before being transplanted into a kidney capsule of a NOD.Cg-Prkdc^scid Il2rg^tm1Wjl/SzJ (NSG) mouse (stock number 005557; The Jackson Laboratory), using methods as previously described for the transplantation of islets (19). Glucose stimulation assay was performed 3 months after transplantation. Mice were deprived of food overnight (12–14 h); water was available ad libitum. Each mouse was injected intraperitoneally with a glucose solution (1 mg/g body weight). Before and half an hour after glucose injection, capillary blood glucose was measured and venous blood samples were collected from the tail and submandibular vein. Human C-peptide concentration in the mouse serum was measured by using an ultrasensitive human C-peptide ELISA kit (Mercodia). Nephrectomy was performed on some mice after human C-peptide was detected in the mouse serum. For ER stress studies, TG was administrated by one dose injection of 1 mg/kg of TG intraperitoneally.

One-way ANOVA was applied for multicomparison among groups. Student t-test (two-tailed) was used to compare pairs of experiments. P_α < 0.05 was considered statistically significant.

Protocols to obtain skin biopsies were approved by the Columbia Institutional Review Board and Embryonic Stem Cell Research Oversight Committees. Human subjects gave signed informed consent. Animal protocols were approved by the Columbia Institutional Animal Care and Use Committee.

We obtained skin biopsies and established skin cell lines from two subjects with Wolfram syndrome designated WS-1 and WS-2. Sequencing of the WFS1 locus revealed that WS-2 is homozygous for a frameshift mutation 1230–1233delCTCT (V412fsX440) and that WS-1 is compound heterozygous for V412fsX440 and missense mutation P724L, both mutations that had previously been reported in Wolfram subjects (1,20). Three additional skin cell lines were obtained from Coriell Research Institute from two siblings with Wolfram syndrome: WS-3 and WS-4 and an unaffected parent (carrier). Both WS-3 and WS-4 are compound heterozygous for the mutations W648X and G695V in the WFS1 protein (1) (Fig. 1A). All Wolfram subjects had childhood-onset diabetes, with the earliest onset at age 2 years for WS-2 and between ages 11 and 13 years for WS-1, WS-3, and WS-4. The relationship of these specific mutations to age of onset of diabetes is unknown. All subjects required treatment with exogenous insulin and had optic atrophy. WS-1 has no history of hearing loss or diabetes insipidus, but optic atrophy was discovered at age 14 years. For WS-2, diabetes insipidus and optic atrophy developed at age 13 years. Progressive visual loss and cognitive disabilities have developed in both WS-1 and WS-2. An ES cell line HUES42 (21) (control-1) and an iPS cell line (control-2) generated from a healthy individual were used as normal controls. DNA sequencing confirmed that these two control cell lines do not carry any coding mutations in WFS1. To control for effects of genetic background, we included cells of the nondiabetic parent heterozygous for the mutation G695V in our analyses (Supplementary Table 1) and genetically rescued the WFS1 locus by expressing a cDNA transgene under the murine stem cell virus promoter.

We generated iPS lines from the four Wolfram subjects and the control subjects using nonintegrating Sendai virus vectors encoding the transcription factors Oct4, Sox2, Klf4, and c-Myc (13). All iPS cell lines were karyotypically normal, expressed markers of pluripotency and differentiated into cell types and tissues of all three germ layers in vitro and after injection into immune-compromised mice (Supplementary Fig. 1). iPS cell lines from Wolfram and control subjects were differentiated into insulin-producing cells using stepwise differentiation into definitive endoderm (SOX17-positive cells), pancreatic endoderm (PDX1-positive cells), and β-cells (C-peptide-positive) (Fig. 1B). Differentiation efficiency of Wolfram cells was similar to controls: after 8 days of differentiation, approximately 80% of all cells expressed PDX1, a marker of pancreatic endocrine progenitors, and after 13 days of differentiation, approximately 20% of all cells expressed C-peptide (Fig. 1C, Supplementary Fig. 2). Immunostaining revealed that WFS1 was specifically expressed in insulin-producing cells but not in glucagon-positive cells (Fig. 1D), which is consistent with the expression pattern reported for mouse islets (5).

To investigate the effects of WFS1 mutations on β-cell function, we quantified insulin mRNA and protein content in Wolfram and control stem cell–derived β-cells. WFS1 deficiency was associated with a 40–50% reduction in insulin mRNA levels compared with controls (Fig. 2A), a 30–40% decrease of insulin protein content (Fig. 2B), and a 30–40% decrease in the number of secretory granules (Fig. 2C and D). Insulin production was restored to levels of control cells by a transgene encoding wild-type WFS1, indicating that WFS1 deficiency, and not other genetic differences, resulted in reduced insulin content (Fig. 2A–D).

To determine the cause of the decreased insulin content, we analyzed the ratio of proinsulin/insulin in β-cells. We found that the proinsulin/insulin ratio in Wolfram β-cells was between 0.4 and 0.55, similar to control cells (0.4–0.47) (Fig. 3A, Supplementary Fig. 3). We next investigated the expression of components of the UPR in Wolfram and control cells. Three branches of the UPR, inositol-requiring protein 1α (IRE1α), protein kinase RNA-like ER kinase (PERK), and ATF6, sense increases in unfolded protein and respond with modulation of cellular, transcriptional, and translational activities (22). It has previously been reported that chronic hyperactivation of IRE1 leads to decreased insulin mRNA and protein level in INS-1 cells (23). Using quantitative PCR and Western blotting, we found that in fibroblasts, iPS cells, and β-cells, components of the three major UPR pathways were increased in Wolfram subject samples in comparison with controls, including spliced XBP-1 (sXBP-1) mRNA, which is downstream of IRE1, ATF4 mRNA, and nuclear ATF6α, p-eIF2α (eukaryotic translation initiation factor-2α) and GRP78 protein (Fig. 3B–E, Supplementary Fig. 4). These differences were amplified by the imposition of experimental ER stress. TG, which impairs protein folding by interfering with calcium homeostasis in the ER (24), caused a greater increase of GRP78 mRNA levels in Wolfram (fourfold) than in control stem cells (twofold) (Supplementary Fig. 4A). A stronger UPR response in Wolfram cells than in control cells is also observed with the application of another ER stress inducer, TM, an inhibitor of N-linked glycosylation (25) (Supplementary Fig. 4B and C). Experimentally induced ER stress also affected ER morphology: the ER was greatly dilated in Wolfram β-cells in the presence of a low dose of TG, while control cells were unaffected (Fig. 3G, Supplementary Fig. 5). Insulin processing was similarly affected; treatment with low doses of TG resulted in the accumulation of proinsulin in Wolfram but not in control cells (Fig. 3A). The upregulation of UPR pathways, including increased sXBP-1 mRNA, a downstream target of IRE-1α, suggests that the UPR response is likely responsible for the reduced insulin content and insulin processing in β-cells.

To determine if preventing the activation of the UPR could restore normal insulin content in Wolfram cells, we generated β-cells in the presence of the chemical chaperone sodium 4PBA during days 9 to 15 of differentiation. 4PBA can assist protein folding and thereby reduce the activity of UPR pathways (26). 4PBA (27,28) and TUDCA (29) reduced GRP78 mRNA levels in Wolfram cells treated with TG (Fig. 3F). Nuclear ATF6α, p-eIF2α protein levels, and sXBP-1 as well as ATF4 mRNA levels were reduced by 30–50% in comparison with no 4PBA vehicle controls (Fig. 3B–E). Strikingly, insulin mRNA levels in Wolfram cells were increased by 1.9-fold and insulin content by 1.5–1.9-fold to levels comparable to those in control cells without 4PBA (Fig. 2A and B). The number of secretory granules in Wolfram β-cells was also substantially increased with the treatment of long-term 4PBA or with the expression of exogenous wild-type WFS1 protein (Fig. 2C and D). When control cells were exposed to the same 7d treatment with 4PBA during β-cell differentiation, no significant increase of insulin production was observed (Fig. 2A and B). Also, insulin processing was normalized by the treatment of 4PBA after exposure to TG (Fig. 3A). These results demonstrate that activation of the UPR mediates the reduced insulin content in WFS1 mutant β-cells. The activation of all three UPR pathways suggests that WFS1 acts upstream of the UPR, likely to maintain ER function under protein folding stress.

To determine whether a specific insulin secretion pathway was affected in Wolfram cells, we exposed them to various insulin secretagogues, including glucose, arginine, potassium, and the cAMP analog, DBcAMP. Others have previously reported that glucose stimulates insulin secretion by ATP generation, resulting in the closing of ATP-sensitive potassium channels and reduction of potassium efflux, which depolarizes the cell, stimulating Ca²⁺ influx and exocytosis of insulin granules (30). Arginine induces insulin secretion by triggering Ca²⁺ influx, without reducing potassium efflux (31). cAMP influences insulin secretion through activation of protein kinase A and/or exchange proteins activated by cAMP (32). Finally, extracellular potassium directly depolarizes the plasma membrane, resulting in the release of insulin granules (33). To assess insulin secretion in response to glucose, we incubated cells in 5.6 mmol/L glucose for 1 h, followed by incubation in 16.9 mmol/L glucose for 1 h. Control and the WFS1 mutation carrier β-cells showed a 1.6- to 1.7-fold increase in C-peptide release in 16.9 mmol/L glucose (vs. 5.6 mmol/L glucose). A similar 1.5- to 1.9-fold increase was seen in the four WFS1 mutant cell lines (Fig. 4A and B). Similarly, arginine, potassium, and DBcAMP increased C-peptide secretion (twofold to fourfold) equally in control and WFS1 mutant cells (Fig. 4A). Therefore, WFS1 mutant β-cells displayed functional responses to secretagogues acting at different points in pathways of metabolic sensing and insulin release comparable to control cells.

We next determined whether WFS1 deficiency affected stimulated insulin secretion under imposed ER stress. When TG-treated cells were exposed to high ambient glucose (16.9 mmol/L), Wolfram cells failed to increase C-peptide secretion, while control β-cells increased C-peptide output by 1.6-fold (vs. 5.6 mmol/L glucose). Incubation with 4PBA prevented the effect of TG on Wolfram β-cells (Fig. 4A, Supplementary Fig. 6). The reduction in stimulated C-peptide secretion by TG was seen with all secretagogues tested. Independent of the secretagogues applied, the chemical chaperone 4PBA prevented the decrease in C-peptide secretion upon application of ER stressor (Fig. 4A). A reduction in stimulated C-peptide secretion was observed for β-cells generated from all four Wolfram subjects but not for the WFS1 mutation carrier or the nonmutant control iPS cell line (Fig. 4B and C, Supplementary Fig. 7). The reduced β-cell function was not specific to TG: a comparable reduction in insulin secretion was also observed in TM-treated Wolfram β-cells upon potassium or glucose stimulation (Fig. 4B and C). Importantly, a wild-type WFS1 transgene reduced sensitivity to the ER stress agent TG, showing a response to both arginine and DBcAMP stimulation comparable to controls (Supplementary Fig. 8).

To determine if the reduction in insulin secretion was due to β-cell death, we quantified the number of insulin-positive cells over 72 h, with or without TG treatment. Insulin cell number remained constant after 72 h incubation with 10nM TG (Supplementary Fig. 9A). We further tested the ER-stress-related cell death marker gene expression, such as CHOP (C/EBP homologous protein, also known as DNA damage-inducible transcript 3 encoded by the DDIT3 gene) (34) and TXNIP (thioredoxin-interacting protein) (35), both proteins involved in ER-stress-dependent apoptosis. A higher increase of CHOP mRNA expression was observed in Wolfram cells compared with control cells after TG treatment for 12 h, but expression level of TXNIP mRNA showed no significant changes in control and Wolfram cells (Supplementary Fig. 9B and C). Therefore, ER stress did not reduce insulin secretion by inducing cell death during the time frame studied but rather by affecting the ability of β-cells to secrete insulin.

Because of the specific expression of WFS1 in β-cells (Fig. 1D) but not in glucagon-expressing cells, we anticipated that WFS1 mutations differentially affect β- and α-cell function. We differentiated Wolfram cells into clusters containing both glucagon- and insulin-expressing cells (Fig. 1D) and stimulated these cells with arginine. As arginine stimulates both endocrine cell types, we were able to assess stimulated hormone secretion in the same cell cluster in the presence and absence of TG. TG treatment reduced arginine-stimulated glucagon secretion in control and WFS1 mutant cells by 28 and 24%, respectively. In contrast, a reduction of stimulated insulin secretion occurred only in WFS1 mutant cells (3% increase in control cells vs. 43% decrease in WFS1 cells) (Fig. 4D). These results show that the insulin secretion phenotypes in WFS1 mutant cells are not due to changes in glucagon release in adjacent cells (36) and demonstrate that WFS1 (which is not expressed in islet α-cells) specifically protects β-cells from the detrimental effects of ER stress.

In vitro studies may not fully recapitulate all relevant molecular cellular circumstances in a systemic physiological environment. The transplantation of β-cells allows testing functionality of β-cells in vivo over a time period of several months. After 12 days of in vitro differentiation, cell culture containing 70–80% PDX1+ cells, were transplanted under the kidney capsule of immune-deficient mice. Human C-peptide was detected 13 weeks post-transplantation in the serum of 13/16 mice transplanted with control cells and 14/20 mice transplanted with Wolfram cells. Basal C-peptide serum levels were comparable for both Wolfram and control HUES42-derived cells (Supplementary Fig. 10A). Human C-peptide was graft derived, as human C-peptide became undetectable in blood 2 days after the removal of the kidney containing the transplanted cells (Supplementary Fig. 10B). Cells contained in the graft coexpressed C-peptide and urocortin 3, which labels functional mature β-cells (37) (Fig. 5A). Upon systemic glucose challenge, Wolfram-derived cells were able to respond to glucose administered intraperitoneally by increasing human C-peptide secretion. However, they displayed significantly reduced responsiveness compared with human islets and β-cells derived from control stem cells (Fig. 5B). We then performed repeated measurement of human C-peptide over a 1-month period, starting from 3 months post-transplantation surgery when the mice were found to show glucose-stimulated human insulin secretion. During this 1-month period, human islets and control grafts remained unchanged in both fasting and glucose-stimulated C-peptide secretion. In contrast, both fasting C-peptide level and glucose responsiveness of Wolfram β-cells further decreased (Fig. 5C and D). To determine the level of ER stress in the transplanted cells, we isolated the grafts and performed immunohistochemistry for ATF6α and CHOP. Both ATF6α and CHOP staining were more intense in Wolfram β-cells, while control β-cells, human islets, as well as the surrounding grafted cells and mouse tissue showed lower intensity of staining (Fig. 5E and F). To test whether ER stress can mediate decreased C-peptide secretion from Wolfram β-cells in vivo, we challenged transplanted mice with TG. Basal C-peptide secretion from Wolfram cells was significantly decreased, while secretion of C-peptide from human islets remained constant (Supplementary Fig. 10C and D).

Here we report the first human cell model of an ER-related disorder, a stem-cell-based model of Wolfram syndrome. This model allowed us to study the consequences of ER stress on β-cell function. β-Cells of Wolfram subjects produce less insulin and have increased activity of three major UPR pathways, including PERK, IRE1, and ATF6. Addition of the chemical chaperone 4PBA reduced levels of UPR signaling pathway molecules and increased insulin content. These results demonstrate that WFS1 protects β-cells from protein folding stress and ER dysfunction, acting upstream of UPR signaling and not by regulating the activity of a particular component of the UPR pathway. Interestingly, low levels of UPR signaling affected insulin content but did not affect insulin processing or stimulated insulin secretion in vitro. However, following imposition of chemical ER stress, insulin processing, ER morphology, and stimulated insulin secretion were greatly affected. These phenotypes observed in vitro were recapitulated in vivo after cell transplantation: Wolfram-derived cells displayed significantly reduced responsiveness to increased circulating glucose, and the levels of immunohistochemical staining of ER-stress-associated protein ATF6α and CHOP were increased in Wolfram implants in comparison with controls, consistent with previous observations in a rodent model (12). Graft function of Wolfram but not control cells decreased over the time frame of 1 month, suggesting that Wolfram cells have a reduced ability to cope with a challenging metabolic environment in vivo, characterized by fluxes of glucose, free fatty acids, and other metabolites. Disease progression in human subjects may follow a similar course, from elevated UPR signaling resulting in reduced insulin content to chronic ER stress and β-cell failure. Our data suggest that unresolved ER stress will ultimately lead to ER dysfunction, reduced processing of insulin, and blunted insulin secretion.

In type 1 diabetes, a decreasing number of β-cells endeavor to meet metabolic demand for insulin, and in most instances of type 2 diabetes, the demand for insulin is increased because of peripheral insulin resistance. β-Cells of type 2 diabetes and type 1 diabetes subjects may possess greater intrinsic ability to increase insulin synthesis in response to metabolic demand than Wolfram β-cells but eventually encounter a similar situation, where metabolic demand requires insulin production at levels inducing a UPR response. If the disparity between demand and production remains unresolved, β-cell demise ensues. Increased expression of ER stress mediators has been observed in the islets of type 1 diabetic mice (38) and humans (39). Activation of ER-stress-associated genes (i.e., PERK and GRP78) has also been observed in the livers of mouse models of type 2 diabetes (40), and ER stress also appears to contribute to β-cell apoptosis in type 2 diabetes patients (41). Reducing the demand for insulin by intensive insulin therapy improves endogenous β-cell function in type 1 diabetes (42), and improving insulin sensitivity by peroxisome proliferator-activated receptor γ inhibitors or by weight loss meliorates type 2 diabetes, in part, because β-cell function is improved (43,44). In the aggregate, these earlier studies and those reported here support a role for ER stress in mediating aspects of the susceptibility and response of β-cells to failure in the context of diabetes.

Common alleles of WFS1 are associated with increased diabetes risk (45), suggesting that our model of β-cell failure in Wolfram syndrome is also relevant to other forms of diabetes. Significantly, our model provides a platform for drug discovery and testing. We found that the chemical chaperone 4PBA is effective at reverting ER-stress-associated phenotypes in β-cells. In addition to insulin therapy, this molecule—or compounds with similar activity—may be useful in preventing or delaying β-cell dysfunction in Wolfram syndrome and possibly other forms of diabetes.

Acknowledgments. The authors are grateful to the research subjects who enabled this research. The authors thank Ellen Greenberg (Naomi Berrie Diabetes Center, Columbia University) for assistance with subject recruitment and study coordination, Kristy Brown (Department of Pathology and Cell Biology, Columbia University) for electron microscope study assistance, and Fumihiko Urano (Washington University School of Medicine) for providing the WFS1 antibody and for helpful discussions.

Funding. This work was supported by the New York Stem Cell Foundation, the Leona M. and Harry B. Helmsley Charitable Trust, the Berrie Foundation Program in Cellular Therapies of Diabetes, the National Institutes of Health (DK-52431, P30-DK-063608), and the Hunter Eastman Scholar Award in Translational Diabetes Research. D.E. is a New York Stem Cell Foundation–Robertson Investigator.

Duality of Interest. No potential conflicts of interest relevant to this article were reported.

Author Contributions. L.S. wrote the manuscript, researched data, and designed research. H.H. researched data, contributed to discussion, and designed research. K.F., H.M., K.W., M.Z., D.J.K., M.F., W.C., and C.L. researched data and contributed to discussion. R.G. reviewed and edited the manuscript. R.L.L. and D.E. reviewed and edited the manuscript and designed research. D.E. is the guarantor of this work and, as such, had full access to all the data in the study and takes responsibility for the integrity of the data and the accuracy of the data analysis.