A Critical Link Between Glucose Toxicity and β-Cell Apoptosis
- 1Department of Medicine, University of Wisconsin, Madison, Wisconsin
- 2Department of Medicine, University of California, Los Angeles, California
- Address correspondence and reprint requests to Anath Shalev, MD, University of Wisconsin-Madison, H4/526 Clinical Science Center, 600 Highland Ave., Madison, WI 53792. E-mail:
OBJECTIVE—In diabetes, glucose toxicity affects different organ systems, including pancreatic islets where it leads to β-cell apoptosis, but the mechanisms are not fully understood. Recently, we identified thioredoxin-interacting protein (TXNIP) as a proapoptotic β-cell factor that is induced by glucose, raising the possibility that TXNIP may play a role in β-cell glucose toxicity.
RESEARCH DESIGN AND METHODS—To assess the effects of glucose on TXNIP expression and apoptosis and define the role of TXNIP, we used INS-1 β-cells; primary mouse islets; obese, diabetic BTBR.ob mice; and a unique mouse model of TXNIP deficiency (HcB-19) that harbors a natural nonsense mutation in the TXNIP gene.
RESULTS—Incubation of INS-1 cells at 25 mmol/l glucose for 24 h led to an 18-fold increase in TXNIP protein, as assessed by immunoblotting. This was accompanied by increased apoptosis, as demonstrated by a 12-fold induction of cleaved caspase-3. Overexpression of TXNIP revealed that TXNIP induces the intrinsic mitochondrial pathway of apoptosis. Islets of diabetic BTBR.ob mice also demonstrated increased TXNIP and apoptosis as did isolated wild-type islets incubated at high glucose. In contrast, TXNIP-deficient HcB-19 islets were protected against glucose-induced apoptosis as measured by terminal deoxynucleotidyl transferase-mediated dUTP nick-end labeling and caspase-3, indicating that TXNIP is a required causal link between glucose toxicity and β-cell death.
CONCLUSIONS—These findings shed new light onto the molecular mechanisms of β-cell glucose toxicity and apoptosis, demonstrate that TXNIP induction plays a critical role in this vicious cycle, and suggest that inhibition of TXNIP may represent a novel approach to reduce glucotoxic β-cell loss.
- ER, endoplasmic reticulum
- INS-LacZ, INS-1 cells overexpressing LacZ
- INS-TXNIP, INS-1 cells with constitutive TXNIP overexpression
- HBSS, Hanks' balanced salt solution
- TUNEL, transferase-mediated dUTP nick-end labeling
- TXNIP, thioredoxin-interacting protein
Type 2 diabetes is a growing public health issue characterized by peripheral insulin resistance and decompensation of the pancreatic β-cells that can no longer keep up with the increased insulin requirements, resulting in hyperglycemia. These elevated glucose levels have detrimental effects on various tissues including the pancreatic β-cell. β-Cell glucose toxicity leads to progressive β-cell dysfunction, impaired insulin gene transcription (1,2), and irreversible β-cell loss by apoptosis (3–14), resulting in a vicious cycle with worsening hyperglycemia. However, the exact molecular mechanisms by which glucose toxicity leads to apoptotic β-cell loss are still not fully understood.
Recently, we identified thioredoxin-interacting protein (TXNIP) as a highly glucose-regulated proapoptotic factor in β-cells (15), suggesting that it may represent a potential mediator of β-cell glucose toxicity. TXNIP binds to and inhibits thioredoxin and thereby can modulate the cellular redox state and promote oxidative stress (16–20). In addition, TXNIP has been shown to exert antiproliferative effects by inducing cell-cycle arrest at the G0/G1 phase (16,21,22), and TXNIP overexpression rendered fibroblasts and cardiomyocytes more susceptible to apoptosis (16,23). Similarly, we found that TXNIP overexpression also induces apoptosis in pancreatic β-cells (15). Moreover, we demonstrated that glucose stimulates TXNIP transcription through a carbohydrate response element in the TXNIP promoter, resulting in elevated TXNIP mRNA expression (15). Together, these findings raised the possibility that TXNIP might play a role in the glucotoxic β-cell death associated with diabetes. The present study was therefore aimed at determining whether glucose and/or diabetes upregulate TXNIP protein levels in vivo and if so how this affects β-cell apoptosis. To further investigate the causal relationship and address the question of whether TXNIP is critical for glucose toxicity–induced β-cell apoptosis, we used TXNIP-deficient primary HcB-19 islets.
RESEARCH DESIGN AND METHODS
All mouse studies were approved by the University of Wisconsin Animal Care and Use Committee, and the National Institutes of Health principles of laboratory animal care were followed. Obese, insulin-resistant, and diabetic BTBR.ob mice (The Jackson Laboratories, Bar Harbor, ME) homozygous for the leptinob mutation were used as a model of type 2 diabetes (24–26). Diabetes was confirmed by blood glucose measurements using a OneTouch Ultra glucometer. Lean and normoglycemic BTBR.lean mice were used as controls. The C3H congenic TXNIP-deficient HcB-19 (HcB) mice harboring a naturally occurring nonsense mutation in the TXNIP gene and the control C3H/DiSnA (C3H) strain have been described previously (27–29). C57BL/6 mice were purchased from The Jackson Laboratory.
Mouse pancreatic islets were isolated by a collagenase digestion procedure as described previously (25,26). In brief, immediately after the mice were killed, pancreata were inflated with 5 ml collagenase solution (0.40 mg/ml type XI collagenase; Sigma, St. Louis, MO) in Hanks' balanced salt solution (HBSS) (Invitrogen, Carlsbad, CA) with 0.02% radioimmunoassay-grade BSA (Sigma) and placed in 25 ml of the same solution, gassed with 95%O2/5%CO2 for 5 min, and vigorously shaken at 37°C for 14 min. After a quick spin, the tissue pellet was washed twice with 10 ml cold HBSS, passed through a 925-micron Spectra mesh filter (Fisher, St. Louis, MO) to remove large debris, and resuspended in 5 ml of 25% Ficoll (type 400-DL; Sigma) prepared with HBSS in a 50-ml conical tube. A total of 2.5 ml of 23, 20.5, and 11% Ficoll were layered carefully on top of each other, and the gradient was centrifuged for 15 min at 800g. Layers above the 25% Ficoll containing the isolated islets were collected, washed with HBSS, and the islets pelleted by a 5-min centrifugation at 800g. To further exclude contamination by exocrine tissue, islets were handpicked under stereomicroscopic observation and used immediately for protein extraction or incubation at low or high glucose. Human pancreatic islets were isolated from brain-dead organ donors under a protocol approved by the University of Wisconsin Institutional Review Board and were a generous gift of Drs. Matthew Hanson and Luis A. Fernandez.
INS-1 cells were grown in RPMI-1640 (Invitrogen) supplemented with 10% fetal bovine serum, 1% penicillin-streptomycin, 1 mmol/l sodium pyruvate, 2 mmol/l l-glutamine, 10 mmol/l HEPES, and 0.05 mmol/l 2-mercaptoethanol. INS-1 cells with constitutive TXNIP overexpression (INS-TXNIP) and control cells overexpressing LacZ (INS-LacZ) were generated and selected as described previously (15). INS-1 cells and isolated HcB-19, C3H, C57BL/6, or human islets were incubated in RPMI supplemented with 10% fetal bovine serum and 1% penicillin-streptomycin and containing 5 or 25 mmol/l glucose for 24 h before protein extracts were prepared or cells were fixed for immunohistochemistry.
Protein extracts were prepared using a lysis buffer containing HEPES (50 mmol/l), Nonidet P-40 (10%), sodium fluoride (100 mmol/l), sodium pyrophosphate (10 mmol/l), EDTA (4 mmol/l), phenylmethanesulphonyl fluoride (1 mmol/l), leupeptin (2 μmol/l), activated sodium orthovanadate (2 mmol/l), and okadaic acid (100 nmol/l). INS-1 cells were grown in T75 flasks and scraped into 0.2 ml of lysis buffer. Isolated primary mouse islets of two animals were pooled and suspended in lysis buffer (20 μl/200 islets). Proteins were separated by 4–20% SDS-PAGE, blotted onto polyvinylidene difluoride membranes, and detected using the following primary antibodies: TXNIP (1:400) (JY2; MBL International, Woburn, MA), monoclonal cleaved caspase-3 (1:200) (Cell Signaling, Boston, MA), and β-actin (1:200) (Abcam, Cambridge, MA) and the following secondary antibodies: anti-mouse IgG (1:5,000) (Amersham, Piscataway, NJ) and anti-rabbit IgG (Bio-Rad, Hercules, CA). Bands were visualized by Lumigen PS-3 detection reagent (Amersham) and quantified by ImageQuant version 5.1 (GE Healthcare Lifesciences).
Immunohistochemistry and terminal deoxynucleotidyl transferase-mediated dUTP nick-end labeling.
For immunohistochemistry and transferase-mediated dUTP nick-end labeling (TUNEL), ∼100 isolated mouse islets were mixed with 15 μl of Affi-Gel Blue Gel (Bio-Rad), fixed in 4% formaldehyde, washed in PBS, and the pellets resuspended in 0.5 ml of warm 2% Difco-agar in an Eppendorf tube and centrifuged for 10 s at 10,000 rpm. After solidification, the agar containing the islet pellet was removed from the tube, trimmed, refixed, and processed in an automated Shandon Citadel 100 machine before paraffin embedding and preparation of 5-μm sections.
For TUNEL, the DeadEnd Fluorometric TUNEL System kit (Promega, Madison, WI) was used according to the manufacturer's instructions, but a permeabilization step was included (5 min in a 1% Triton X-100 PBS solution). β-Cells were visualized by insulin staining using guinea pig anti-insulin antibody (Zymed, San Francisco, CA) and Cy3-conjugated anti-guinea pig IgG (1:500; Jackson ImmunoResearch, Westgrove, PA). The Vectashield with 4,6-diamidino-2-phenylindole mounting solution (Vector, Burlingame, CA) was used for visualization of nuclei. β-Cell proliferation was assessed by staining 10-μm pancreatic sections for Ki67 (1:200; Abcam).
Whole-pancreas insulin content.
Sixteen-week-old male HcB-19 (n = 5) and C3H control mice (n = 4) were killed after a 4-h fast, and their whole-pancreas insulin content (μg/pancreas) was assessed by acid-ethanol extraction, and insulin enzyme-linked immunosorbent assay was used as a measure of β-cell mass.
Insulin secretion and glucose-induced insulin secretion of isolated C3H and HcB-19 islets were assessed after an overnight incubation at 5 mmol/l glucose as described previously (30,31). All experiments were performed in triplicates using three islets per tube.
Cytochrome C release.
To obtain cytosolic and mitochondrial cell fractions, cells from two T-75 flasks per sample were trypsinized and collected by centrifugation at 1,000g for 2 min. Cells were then washed with PBS and the cell pellet resuspended in 200 μl of buffer A (20 mmol/l Hepes-KOH, pH 7.5; 10 mmol/l KCl; 1.5 mmol/l MgCl2; 1 mmol/l EGTA; 1 mmol/l dithiothreitol; 250 mmol/l sucrose; 100 mmol/l phenylmethylsulfonyl fluoride; 1 μg/ml pepstatin A; 2 μg/ml leupeptin; and 2 μg/ml aprotinin). The homogenate was then centrifuged at 1,000g for 10 min at 4°C, and the supernatant containing the cytosolic and mitochondrial fractions was centrifuged again for 15 min at 10,000g at 4°C. The resulting supernatant contained the cytosolic fractions, and the pellet contained the mitochondrial fractions. The cytosolic fractions were boiled in SDS sample buffer and frozen at −80°C until further analysis. Pellets containing mitochondria were treated with buffer B (1 × PBS; 1% Nonidet P-40; 0.5% sodium deoxycholate; 0.1% SDS; 250 mmol/l sucrose; 20 mmol/l Tris HCl, pH 7.4; 1 mmol/l dithiothreitol; and protease inhibitors) and were incubated on ice for 20 min. The lysate was centrifuged at 10,000g for 30 min at 4°C. The pellet was solubilized in buffer C (300 mmol/l sucrose; 1 mmol/l EGTA; 20 mmol/l MOPS, pH 7.4; 0.5 mg/ml BSA; and protease inhibitors), and the resulting mitochondria-enriched fractions were boiled in SDS sample buffer and stored at −80°C until further use. Cytochrome C protein levels in the mitochondrial and cytosolic fractions were determined by Western blotting using a mouse monoclonal cytochrome C antibody (1:500; Santa Cruz Biotechnology, Santa Cruz, CA) and anti-mouse IgG (1:2,000; Amersham, Piscataway, NJ).
Quantitative real-time RT-PCR.
RNA was extracted using Trizol, converted to cDNA with the First Strand cDNA synthesis kit (Roche), and analyzed on a Prism 7000 Sequence Detection System (Applied Biosystems). BiP was amplified using the forward primer 5′-ACGTCCAACCCGGAGAACA-3′ and the reverse primer 5′-TTCCAAGTGCGTCCGATGA-3′ and ChOP with 5′-TGGCACAGCTTGCTGAAGAG-3′ and 5′-TCAGGCGCTCGATTTCCT-3′, respectively. Total TXNIP was measured using primers recognizing both human and rat TXNIP (forward: 5′-ACAGAAAAGGATTCTGTGAAGGTGAT-3′, reverse: 5′-GCCATTGGCAAGGTAAGTGTG-3′). All samples were corrected for the 18S ribosomal subunit (Applied Biosystems) run as an internal standard.
To calculate the significance of a difference between two means, we used two-sided Student's t tests. A P value of <0.05 was considered statistically significant.
TXNIP protein levels and cleaved caspase-3 expression are elevated in response to glucose in INS-1 β-cells.
We previously found that glucose induces TXNIP transcription. To now determine whether the observed glucose effects are also translated into differential expression of TXNIP at the protein level, we performed Western blot experiments using INS-1 β-cells incubated at low (5 mmol/l) or high (25 mmol/l) glucose for 24 h. We observed that incubation at high versus low glucose induced TXNIP protein expression 18-fold (Fig. 1). Interestingly, we found that these elevated TXNIP protein levels were accompanied by a 12-fold increase in cleaved (activated) caspase-3 (Fig. 1C), suggesting increased apoptosis.
These findings are consistent with our previous demonstration of glucose increasing β-cell TXNIP mRNA levels (15,32) and the observation that TXNIP overexpression promotes β-cell apoptosis (15,30) as well as with the proapoptotic properties of TXNIP described in extrapancreatic tissues (16,23). They also suggest that TXNIP-mediated β-cell apoptosis does not require constitutive overexpression of TXNIP but rather that the glucose-induced increase in endogenous TXNIP is sufficient for this effect. This raised the possibility that TXNIP might be involved in the pathophysiology of type 2 diabetes and the associated β-cell loss.
Diabetic mice demonstrate increased levels of TXNIP and cleaved caspase-3 in their pancreatic islets.
To test whether diabetes alters in vivo TXNIP expression in pancreatic islets, we analyzed islets isolated from obese, insulin-resistant, and diabetic BTBR.ob mice harboring the leptinob mutation as a model of type 2 diabetes (24–26). These analyses revealed that TXNIP protein levels were elevated eightfold in islets of obese diabetic BTBR.ob mice compared with lean normoglycemic controls (BTBR.lean), and this increase in TXNIP was again accompanied by an equal rise in cleaved caspase-3 levels (Fig. 2). These data are in agreement with the elevated TXNIP mRNA expression observed in islets of nonobese, insulin-resistant C57BL/6.azip mice as another model of diabetes (15) and further support an in vivo role of TXNIP in diabetes and β-cell death.
However, we also wanted to assess the causal relationship between glucose-induced TXNIP expression and β-cell apoptosis and determine whether TXNIP is critical for this effect. To this end, we studied TXNIP-deficient HcB-19 mice. HcB-19 mice are an inbred congenic C3H mouse strain (33,34) that harbors a spontaneous inactivating nonsense mutation in exon 2 at codon 97, resulting in dramatically reduced TXNIP mRNA and protein levels (29).
Glucose induces TXNIP expression and apoptosis in primary islets.
To determine the role of TXNIP in glucose toxicity–mediated β-cell apoptosis, we first analyzed wild-type islets with normal TXNIP expression isolated from control C3H mice. In analogy to the INS-1 cell experiments, we incubated isolated islets at low or high glucose for 24 h and then assessed them for the expression of TXNIP, cleaved caspase-3, and by TUNEL. Again, we observed that incubation at high glucose resulted in elevated TXNIP protein levels and increased apoptosis, as measured by the sevenfold increase in cleaved caspase-3 (Fig. 3) and the ninefold higher percentage of TUNEL-positive β-cells (Fig. 4) compared with C3H islets incubated at low glucose. We also obtained very similar findings in islets isolated from C57BL/6 mice as well as in human islets (Fig. 5). In addition, incubation of human islets at 25 mmol/l glucose for 24 h also led to an ∼2-fold increase in TXNIP protein levels and a >10-fold increase in cleaved caspase-3.
TXNIP deficiency protects against glucose toxicity–induced β-cell apoptosis.
In contrast, parallel experiments using isolated islets of TXNIP-deficient HcB-19 mice revealed no increase in TXNIP expression (as expected) but interestingly also failed to demonstrate any increase in cleaved caspase-3 (Fig. 3) or TUNEL-positive β-cells in response to glucose (Fig. 4). These findings strongly suggest that TXNIP expression is critical for the increase in β-cell apoptosis observed in response to high glucose exposure and provide direct evidence for the protective role of TXNIP deficiency against β-cell glucose toxicity.
To address the issue of whether other factors in the mutant HcB-19 islets may have contributed to the observed protection, we repeated the experiments using isolated islets of mice with β-cell–specific deletion of TXNIP created by the Cre-loxP system and of control lox/lox littermates. While incubation at high glucose led again to a significant increase in TUNEL-positive β-cells in the control islets (P = 0.001) similar to C3H, C57BL/6, and human islets, this effect was completely blunted in islets from β-cell–specific TXNIP knockout mice. These findings confirm the results obtained with the HcB-19 islets and demonstrate that it is specifically the lack of TXNIP that protects β-cells against glucose toxicity–induced apoptosis.
To further investigate the contribution of TXNIP to β-cell loss in vivo, we compared the β-cell mass in TXNIP-deficient HcB-19 and control C3H mice. Interestingly, we found that functional β-cell mass was more than twofold higher in the TXNIP-deficient mice as indicated by a whole-pancreas insulin content of 71.2 ± 1.8 μg/pancreas in HcB-19 mice compared with 35.0 ± 3.9 μg/pancreas in control C3H mice (P = 0.001). At the same time, TXNIP deficiency did not seem to affect β-cell proliferation, as no difference in the number of Ki67-positive β-cells was observed between HcB-19 and C3H pancreata in these initial experiments (data not shown). Together with our findings of TXNIP-induced β-cell apoptosis, this suggests that the net increase in β-cell mass observed in response to TXNIP deficiency was primarily due to a decrease in β-cell apoptosis.
TXNIP deficiency does not alter islet insulin secretion.
To assess whether TXNIP deficiency also affects β-cell function, we performed insulin secretion studies using isolated islets from HcB-19 and C3H mice. The results of these experiments demonstrated that basal and glucose-stimulated insulin secretion remained unchanged in TXNIP-deficient islets, suggesting that TXNIP does not interfere with normal islet function (Table 1).
TXNIP induces the intrinsic mitochondrial pathway of apoptosis.
We demonstrated that TXNIP deficiency protects β-cells against glucose-induced cell death and that induction of TXNIP promotes β-cell apoptosis, but the mechanisms involved have remained unknown. Major mechanisms leading to apoptosis consist of the extrinsic pathway activated by extracellular signals and mediated by death receptors and the intrinsic pathways mediated by mitochondrial damage and/or endoplasmic reticulum (ER) stress. As the extrinsic pathway is unlikely to be involved in TXNIP-mediated apoptosis, we focused on the mitochondrial and the ER stress pathways, both of which have been implicated in pancreatic β-cell death (35).
The ER stress–mediated pathway involves depletion of ER calcium stores, accumulation of unfolded proteins, and a stress response including upregulation of ER chaperones such as BiP. Severe or persistent ER stress further activates the apoptosis cascade, which includes upregulation of transcription factors such as ChOP and activation of caspase-12.
In the case of mitochondria-mediated apoptosis, the apoptotic stimulus leads to disequilibrium of proapoptotic Bax and antiapoptotic Bcl-2 and disruption of the mitochondrial membrane potential resulting in release of cytochrome C into the cytosol. This represents a hallmark of this pathway and activates caspase-9.
Both pathways converge at the level of caspase-3 activation, which we consistently observed in our TXNIP studies. To determine which of these pathways is mediating the TXNIP effects, we now used stably transfected INS-TXNIP or INS-LacZ as a control and measured markers of mitochondrial or ER stress–mediated apoptosis.
In control cells, cytochrome C was practically exclusively localized to the mitochondria as expected, whereas INS-TXNIP cells showed a dramatic release of cytochrome C into the cytosolic fractions (Fig. 6A and B). In contrast, measurements of ER stress markers BiP and ChOP failed to demonstrate any increase in the INS-TXNIP cells (Fig. 6C and D) despite proven TXNIP overexpression in the same samples (Fig. 6E). Together, these results suggest that TXNIP activates primarily the mitochondrial pathway of apoptosis. This notion is further supported by our previous observation of increased Bax–to–Bcl-2 ratio and activated caspase-9 in response to TXNIP (15).
The results of the present study reveal for the first time that a protein (TXNIP) is essential for glucose toxicity–induced β-cell apoptosis. While the effects of glucose toxicity on β-cell dysfunction and death have been described extensively (1–14), the molecular mechanisms involved have remained largely elusive. In regard to β-cell dysfunction, small heterodimer partner has recently been identified as a factor inhibiting insulin gene transcription in response to glucose toxicity in INS-1 cells (36) but was not reported to have any effects on β-cell death.
In the present study, we have identified TXNIP as a critical factor mediating glucose toxicity–induced β-cell death and have elucidated the pathways by which TXNIP induces β-cell apoptosis. We found that TXNIP overexpression leads to activation of the intrinsic mitochondrial pathway of apoptosis, while ER stress–mediated processes of cell death remained unaffected by TXNIP (Fig. 6). These findings not only shed new light on the role of TXNIP in β-cell biology and the mechanisms involved but also identify TXNIP as a potential target to interfere with the deleterious effects of glucose toxicity. Such modification could help prevent β-cell apoptosis and the gradual β-cell loss that characterizes type 2 diabetes and ultimately makes type 2 diabetic patients require daily insulin injections. In fact, we found that TXNIP reduction mediates the antiapoptotic effects of exenatide, an antidiabetes drug recently approved for type 2 diabetes (37). The idea of TXNIP deficiency potentially enhancing β-cell mass is further supported by the phenotype of the TXNIP-deficient HcB-19 mice that, aside from elevated plasma triglycerides and ketone bodies, includes hyperinsulinemia and hypoglycemia (27,28). Recent work (38) suggests that lack of TXNIP may cause impaired hepatic glucose production, which could lead to hypoglycemia. However, since we have found that TXNIP induces β-cell apoptosis, it is also possible that lack of TXNIP may slow the natural process of β-cell death and turnover, lead to accumulation of β-cells, and result in increased basal insulin production, which would contribute to the observed hypoglycemia. Indeed, our initial results now demonstrate significantly elevated whole-pancreas insulin content in TXNIP-deficient HcB-19 mice compared with C3H controls, indicating increased pancreatic β-cell mass. These findings strongly support the importance of TXNIP not only as a factor conferring glucose toxicity–induced β-cell apoptosis but also as a novel protein controlling overall pancreatic β-cell loss in vivo.
In the context of diabetes treatment, lowering TXNIP expression may also have beneficial effects in tissues other than pancreatic β-cells, where it again may protect against glucose toxicity. TXNIP expression was found to be increased in human aortic smooth muscle cells in response to incubation at high glucose, and diabetic rats had elevated vascular TXNIP levels (39). Moreover, overexpression of TXNIP induced apoptosis in cardiomyocytes (23) and proliferation of smooth muscle cells (21), suggesting that controlling TXNIP expression might help reduce cardiovascular risk and morbidity in patients with diabetes. In addition, a recent human study (40) demonstrated that TXNIP regulates glucose uptake in adipocytes and skeletal muscle and suggested that TXNIP might play a role in the pathogenesis of type 2 diabetes by altering glucose homeostasis. Decreased TXNIP expression might therefore also enhance glucose uptake and clearance in peripheral tissues and thereby further improve glucose control.
In in vitro experiments, transfection and constitutive TXNIP overexpression has been shown to reduce thioredoxin activity (23), raising the possibility that the opposite might also be true and that the effects of TXNIP deficiency might be mediated by activation of thioredoxin. However, more recent studies using TXNIP-deficient HcB-19 mice revealed no difference in thioredoxin protein levels and no increase in thioredoxin activity compared with control mice (28). This suggests that other thioredoxin-independent pathways might be involved in the protective effects of TXNIP deficiency observed in our experiments using HcB-19 islets.
Taken together, the results of the present study have revealed TXNIP as a critical mediator of glucose toxicity–induced β-cell apoptosis. Moreover, they have demonstrated that β-cell TXNIP protein levels are dramatically induced in response to glucose and that TXNIP expression is elevated in islets of different mouse models of diabetes. This suggests that TXNIP may play an important role in diabetes progression and the associated decline in β-cell mass. Controlling TXNIP expression may therefore represent a novel approach to protect pancreatic β-cells from progressive destruction and to preserve a sufficient amount of insulin-producing β-cell mass in patients with type 2 diabetes.
This work was supported by American Diabetes Association Grants 7-03-JF-37 and 7-07-CD-22 and Juvenile Diabetes Research Foundation Grant 1-2007-790 to A.S.
We thank Anna Szabo for technical assistance and Dr. Susan Bonner-Weir for helpful suggestions with regard to the islet-embedding technique.
Published ahead of print at http://diabetes.diabetesjournals.org on 28 December 2007. DOI: 10.2337/db07-0715.
The costs of publication of this article were defrayed in part by the payment of page charges. This article must therefore be hereby marked “advertisement” in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.
See accompanying commentary, p. 797.
- Received May 25, 2007.
- Accepted December 23, 2007.