Sebastian Friedrich Petry
Lia Mingzhe Sun- Clinical Research Unit, Center of Internal Medicine, Justus Liebig University, Giessen, Germany
Histomorphological and functional alterations in pancreatic islet composition directly correlate with hyperglycemia severity. Progressive deterioration of metabolic control in subjects suffering from type 2 diabetes is predominantly caused by impaired beta-cell functionality. The glutaredoxin system is supposed to wield protective properties for beta-cells. Therefore, we sought to identify a correlation between the structural changes observed in diabetic pancreatic islets with altered glutaredoxin 5 expression, in order to determine an underlying mechanism of beta-cell impairment. Islets of db/db mice presenting with uncontrolled diabetes were assessed in terms of morphological structure and insulin, glucagon, and glutaredoxin 5 expression. MIN6 cell function and glutaredoxin 5 expression were analyzed after exposure to oleic acid and hypoxia. Islets of diabese mice were marked by typical remodeling and distinct reduction of, and shifts, in localization of glutaredoxin 5-positive cells. These islets featured decreased glutaredoxin 5 as well as insulin and glucagon content. In beta-cell culture, glutaredoxin 5 protein and mRNA expression were decreased by hypoxia and oleic acid but not by leptin treatment. Our study demonstrates that glutaredoxin 5 expression patterns are distinctively altered in islets of rodents presenting with uncontrolled diabesity. In vitro, reduction of islet-cell glutaredoxin 5 expression was mediated by hypoxia and oleic acid. Thus, glutaredoxin 5-deficiency in islets during diabetes may be caused by lipotoxicity and hypoxia.
1. Introduction
Type 2 diabetes mellitus is hallmarked by deprivation of the microarchitecture of pancreatic islets and progressive loss of beta-cells due to gluco- and lipotoxicity as well as a chronic state of inflammation (1). In particular, lipotoxicity, as mediated by free fatty acids, is a pivotal pathogenetic factor in type 2 diabetes as it induces pronounced insulin resistance (2) concomitant with significant impairment of insulin secretion (3). Free fatty acids mediate beta-cell death by induction of ER stress (4) and ROS production (5). During high metabolic activity, beta-cells further suffer from a hypoxia-like condition (6), which exhibits substantial damage to its secretory apparatus (7). However, the islets of Langerhans broadly express members of the glutaredoxin (Grx) system (8). These proteins are mainly involved in redox regulation of cellular processes and biogenesis of iron–sulfur proteins. Glutaredoxins (Grxs) are assumed to wield protective properties. Mammals express four Grxs classified as mono- or dithiol Grx dependent on the number of cysteine residues in their active center.
Dithiol oxidoreductases Grx1 and 2 are major actors in thiol-disulfide exchange (9–11). They exercise control over their targets by reversible posttranslational de-glutathionylation of cysteine residues in dependence of glutathione reductase and glutathione. Monothiol Grx3 and 5 have no known catalytic activity. They are essential for biogenesis of proteins containing iron–sulfur clusters (12, 13). Mitochondrial Grx5 is directly involved in the composition of iron–sulfur clusters and thereby essential for mitochondrial, as well as cytosolic iron–sulfur proteins, which are essential for cell function (14). Grx5-deficiency results in elevated susceptibility to oxidative and osmotic stress together with cellular iron overload in yeast (14, 15). In zebra fish lacking Grx5, these pathologies occur together with anemia (16). The relevance of Grx5 for unimpaired heme biosynthesis and iron homeostasis is also apparent in human erythroblasts. An example of the effects of Grx5-deficiency was demonstrated in a patient suffering from defective homozygous GLRX5 mRNA-splicing. This patient presented a distinct phenotype including diabetes mellitus mediated by pancreatic iron overload, indicating the crucial role of Grx5 for unimpaired glucose metabolism (17).
Rodents feature a defined composition of the islets of Langerhans. Predominantly, islets consist of insulin-producing beta- and glucagon-producing alpha-cells. The vast majority of beta-cell mass is located in islet center, while alpha-cells are located in islet periphery, together with delta-, gamma- and epsilon cells (18, 19). In humans, cells are distributed randomly throughout islets (20). It is well accepted that disruption of physiological islet cell compositions occurs in diabetes and has remarkable functional impact (21, 22). Apart from apoptosis, beta-cell loss involves dedifferentiation (23–25) and autophagocytosis, where by the islets undergo remodeling (26, 27). However, the exact mechanisms underlying islet remodeling are not entirely understood and apart from documented expression of Grxs in the islets of Langerhans there is little knowledge about their significance for islet physiology. Despite alpha-cell dysfunction in diabetes mellitus being well known in human subjects and rodents (28, 29), there are no publications addressing Grx expression in glucagon-producing cells. However, data indicate that in contrast to beta-cells, alpha-cells are well-provided with antioxidant enzymes (30).
The aim of this study was to determine whether; (I) islets of db/db mice presenting with uncontrolled diabetes differ qualitatively and quantitatively from lean, leptin-susceptible wild types in terms of Grx5 expression, (II) changes in islet Grx5 protein pattern correlate with structural alterations and shifts in the cellular composition of the islets of Langerhans, (III) leptin action can be delineated from changes in glutaredoxin expression in vitro, and (IV) hypoxia and lipotoxicity have an effect on beta-cell Grx5 expression.
We report reduced Grx5 content in islets, loss of insulin content, and loss of glucagon content in pancreases of db/db mice presenting with uncontrolled diabesity in comparison to lean, non-diabetic C57BL/6 littermates. Islet Grx5 patterns were associated with a reduction of structural complexity of islets. We also describe novel data for a connection between Grx5 and beta-cell insulin secretion capacity in vitro. Changes in beta-cell Grx5 content were shown to be independent from leptin-resistance but were dependent on hypoxia and oleic acid in a dose-dependent manner. This is the first report of distinct histomorphological alterations of islet Grx5 expression patterns during uncontrolled rodent diabesity in context with altered islet composition and a possibly lipotoxicity-mediated loss of beta-cell Grx5 expression.
2. Materials and Methods
2.1. Animal Model
15 male BKS(D)-Leprdb/JOrlRj (db/db) mice and 12 male C57BL/6NRj (C57) mice were acquired at the age of 10 weeks from Janvier Labs and were given 2 weeks to adapt to local animal facility. Number of required mice was calculated regarding manifestation rate of diabetes according to our previous study with type I error of 0.05 and type II error of 0.2. Housing conditions involved room temperature of 22 ± 0.5°C, 12 h light/dark cycle, 60% humidity, and tap water and standard diet pellet food (Altromin, Lage, Germany) ad libitum in individually ventilated cages in groups of five mice in accordance with institutional guidelines. Mice were sedated by isoflurane (5%). Thereafter, pancreas retrieval for histological studies was carried out at 12 or 13 weeks of age for db/db animals and 12 or 14 weeks of age for controls as diabetic animals were symptomatic and could thus not be kept for a prolonged period. Respective time points were pooled for both groups.
2.2. Histochemistry and Immunohistochemistry
Light microscopy was used for detection of insulin (Dako, Hamburg, Germany) and primary assessment of islet morphology. Organs were fixated with 3.5–3.7% formaldehyde, rinsed with 70% ethanol, and stored overnight. Embedding was carried out with paraffin after treatment in ascending alcohol series. Prior to staining, paraffin was removed using terpene (Roti-Histol, Roth, Karlsruhe, Germany) and descending alcohol series. Slides were washed with Tris and blocked with 1% goat serum for 20 min. Primary antibodies diluted in 1% goat serum dissolved in TBS containing 0.3% Triton X-100 (0.3% PBST) were applied overnight at 4°C. Secondary antibodies in 5% mouse serum were applied thereafter for 1 h at room temperature. Fuchsine red staining was used in order to visualize insulin. Staining progress was observed with light microscope and stopped after 1 min in Tris. Staining procedure was finished by counterstaining with hemalum–eosin 10% for 1 min (hemalum) and 5 min (eosin) before preservation and conservation with VectaMount (Vector Laboratories, Burlingame, CA, USA).
2.3. Immunofluorescence
Immunofluorescent staining was used for detection of insulin (Dako, Hamburg, Germany), Glucagon (Novus Biologicals, USA), and Grx5 (kindly provided and validated by Prof. Lillig/Dr. Hanschmann as described in Ref. (31)). Organs were stored overnight in PBS supplemented with 18% sucrose solution, embedded in cryoblock embedding medium (Biosystems, Nunningen, Switzerland) and frozen at −80°C. Organs were sectioned using Leica Crysostat CM1850 (Leica, Wetzlar, Germany) in order to acquire slides of 7 µm thickness. Frozen tissue was fixated with Zamboni (paraformaldehyde in picric acid and PBS as described in Ref. (32)) for 15 min. Slides were washed with Tris-buffer and blocked with 1% donkey serum dissolved in 0.3% TBST for 20 min. Incubation with primary antibodies diluted in 1% donkey serum dissolved in 0.3% PBST took place overnight at 4°C. Secondary antibodies in 5% mouse serum were applied for 1 h at room temperature. Nuclei were stained with Hoechst (Calbiochem, Darmstadt, Germany) in 0.1% TRIS buffer pH 7.6 and samples were preserved with ProLong Gold (Invitrogen, Karlsruhe, Germany).
Extracted pancreases were sectioned entirely. Manual optical assessment for quality was employed, i.e., slides with damaged structure were rejected. Multiple inclusion of the same islets was avoided by maintaining an interval of 140 µm between slides used for analysis and by manual comparison of islets. Appropriate comparability of immunohistological staining was achieved by preparation in batches. Slides were screened entirely, all islets were included. Successful staining of target antigen and avoidance of extensive background staining was verified by comparison against samples prepared without the respective primary antibody.
2.4. Measurement of Islet Area and Quantification of Fluorescent Signals
Images were taken with Leica Application Suite v 3.8.0 using digital microscope camera DFC 420 C (Leica, Wetzlar, Germany). Analysis of islet area and quantification of fluorescent signal of insulin, glucagon, and Grx5 was employed using custom scripts for ImageJ (Wayne Rasband, National Institutes of Health, USA) as described before (33). Briefly, ImageJ was calibrated to match image scale. Single islets were optically selected. Exact islet area was identified using combined overlay images (staining of nuclei, insulin, and glucagon). Islet region was carefully tagged manually by use of freehand selection according to outline of insulin and glucagon staining and typical clusters of stained nuclei. Area of selection was measured, and ROI of identified islets were saved for following analysis.
Absolute area of insulin, glucagon, and Grx5 staining per islet was acquired by applying a threshold value to previously saved ROI. Threshold value was manually adapted to limit selection to staining of the respective antibody. Area of selection was measured and ROI were saved for analysis of fluorescent intensity. Relative area of the respective target antigen per islet was normalized to respective islet area to achieve better comparability between islets of different area. As third parameter of staining area quantification, absolute Grx5 area was set in relation to absolute insulin area for every islet to correlate islet Grx with insulin content.
Quantification of fluorescent intensity of insulin, glucagon, and Grx5 as quantification of respective protein content was obtained by measuring mean fluorescent intensity in the previously identified ROI for areas stained by respective antibodies. Therefore, images were normalized by removing background using slides without primary antibodies and converted to gray scale. Fluorescent intensity was measured in emitted fluorescence and given in mean gray values ranging from 0 (0%) to 255 (100%) and normalized against islet extent to achieve better comparability between islets of different area.
Number of Grx5-positive cells per islet was quantified by manually counting all nuclei per islet and identifying those presenting Grx5 staining. Results were given in percentage of cells displaying Grx5 fluorescence.
For each analysis mean of three individual runs was calculated to limit influence of manual selection of ROI and adaption of threshold values.
2.5. Cell Culture and Protein Analysis
Mouse insulinoma cells 6th subclone (MIN6 cells) cell line was obtained from Dr. Sigurd Lenzen (Institute of Clinical Biochemistry, Hannover Medical School, Hannover, Germany) (34) (originally from Dr. Miyazaki, Institute for Medical Genetics, Kumamoto University Medical School, Japan (35)) and cells were routinely maintained in Dulbecco’s modified Eagle medium (DMEM, Life Technologies, Darmstadt, Germany) containing 25 mM glucose, supplemented with 10% fetal calf serum (biowest, Nuaillé, France), 2 mM l-glutamine, 25 mM Hepes (Biochrom, Berlin, Germany), 285 µM 2-mercaptoethanol (Life Technologies, Darmstadt, Germany), and 1% penicillin/streptomycin (Life Technologies, Darmstadt, Germany). Subculture and maintenance were performed as reported repeatedly in publications from our group (36, 37). MIN6 cells presented in this study were at passages 50-60. We compared earlier passage cells (P < 30) and they did not differ in normal glucose stimulated insulin secretion (GSIS) from P > 30 (data not shown). All assays used MIN6 cells grown to 70-80% confluence unless otherwise stated.
Cells were cultured at 37°C and 5% CO2 and split by trypsinization. Washing was done with PBS before adding 0.5% Trypsin-EDTA (Gibco, Darmstadt, Germany) solution. Detachment was carried out by dilution with DMEM and centrifugation for 4 min at 1,200 RPM before seeding into new flasks.
For leptin cultivation, prior to analysis recombinant mouse leptin (R&D, Wiesbaden, Germany) was applied for 2 and 48 h, respectively. Leptin was pre-diluted to 0.1% in 20 mM Tris–HCl, pH 8.0. Concentrations of 0, 0.075, 0.45, and 2 ng/ml were applied. For fatty acid treatment, oleic acid was applied for 24 h under normoxic and hypoxic (2% O2) atmosphere, respectively. Concentrations of 0, 0.5, and 0.75 mM were applied, respectively. Lysates and supernatant was collected for ELISA/PCR analysis.
Protein expression for insulin and Grx5 was measured in MIN6 cell lysates and supernatant. Prior to lysis, 1 ml supernatant was extracted before cells were washed in ice-cold PBS. Cells were incubated on ice for 20 min in NP-40 lysis buffer (United States Biological, Swampscott, USA). Supernatant was gathered by centrifugation for 20 min at 1,200 RPM. Insulin (DRG Instruments GmbH, Marburg, Germany) and Grx5 (CUSABIO Biotech, Wuhan, China) content was analyzed using ELISA technique. As Grx5 concentration exceeded largest measured standard (1,609.05 pg/ml) at 48 h leptin treatment, data were extrapolated. As absorbance in ELISA reached a plateau, it has to be noted that Grx5 protein level at 2 ng/ml leptin treatment was omitted for analysis.
Cell viability was assessed by Vybrant MTT Cell Proliferation Assay Kit following manufacturer’s instructions (Molecular Probes, Inc., Waltham, MA, USA).
2.6. RNA Isolation, cDNA Synthesis, and qRT-PCR
MIN6 cell RNA was extracted using RNeasy Plus Micro Kit (Qiagen, Düsseldorf, Germany). Total RNA concentration was determined by OD260 nm method using NanoDrop 1000 spectrophotometer (Thermo Scientific, Schwerte, Germany). SuperScript III Reverse Transcriptase kit (Invitrogen, Darmstadt, Germany) was employed to synthesize cDNA. qRT-PR was carried out on real-time PCR System StepOnePlus (Applied Biosystems). PCR included 615 s of activation/denaturation at 95°C and 40 cycles of annealing and elongation (95°C, 30 s each). Primer (Invitrogen, Darmstadt, Germany) concentration for qRT-PCR was 20 pM. Sequences were as follows:
beta-actin (housekeeping in leptin culture):
fwd CGT GAA AAG ATG ACC CAG ATC A, rev CAC AGC CTG GAT GGC TAC GT;
rpl32 (housekeeping in oleic acid culture):
fwd GGA GAA GGT TCA AGG GCC AG, rev GCG TTG GGA TTG GTG ACT CT;
Grx5:
fwd GAA GAA GGA CAA GGT GGT GGT CTT C, rev GCA TCT GCA GAA GAA TGT CAC AGC
Relative mRNA expression values were obtained by normalizing CT values of the target genes in comparison with CT values of the housekeeping gene using the delta-CT method.
2.7. Statistical Analysis
Statistical analysis was performed using Graph Pad Prism 5 (GraphPad Software, San Diego, CA, USA) using Mann–Whitney test and two-way ANOVA as appropriate. Data are given as mean values ± SEM, with n denoting the number of experiments unless otherwise indicated. A p-value < 0.05 was considered significant.
3. Results
3.1. Uncontrolled Diabesity on the Genetic Background of the db Mutation
Obese homozygous leptin-resistant db/db mice were utilized for comparison with lean wild-type C57BL/6 animals as the db strain is typically presenting a strong phenotype of diabesity. Homozygotes featured uncontrolled diabetes mellitus with polyuria and weight loss exhibiting significantly (p < 0.0001) higher blood glucose levels than their lean, non-diabetic littermates. Mean blood glucose value was 471 mg/dl and thus 2.6-fold higher than in controls whose average blood glucose level was 179 mg/dl (Figure 1A). Furthermore, a distinct phenotype of rodent obesity was still apparent despite beginning weight loss in db animals. Average body weight was 52 g in db/db animals in comparison to 29 g in controls (p < 0.0001, Figure 1B).
Figure 1. Blood glucose level and body weight of db/db and C57BL/6 mice. (A) Blood glucose level of db/db and C57BL/6 mice. (B) Body weight of db/db and C57BL/6 mice. Values are mean ± SEM (n = 12–15 mice), black bars represent db/db mice, white bars represent C57BL/6 mice, *** denotes p < 0.0001.
3.2. Loss of Islet Structure and Elevated Islet Area in Rodent Diabesity
To relate the phenotype of uncontrolled diabetes to histomorphological alterations, islet structure was assessed histologically. Light microscopy was used as it allowed for easier discrimination between endocrine and exocrine tissue. Analysis revealed marked differences between islets of diabetic db/db mice and non-diabetic C57BL/6 controls. Pancreases of db animals contained two types of islets: small deformed ones with lost demarcation to exocrine tissue (Figure 2A) as well as a vast number of remarkably extensive islets (Figure 2B). In contrast, C57 islets were clearly defined from exocrine tissue and presented a notably lower variability of islet size (Figure 2C). The optical impression of elevated islet extent was confirmed by quantification of islet area using stained slides. Despite high variability, islets of db/db mice were significantly larger (p < 0.05) than C57 islets (Figure 2D), on average by 1.5-fold.
Figure 2. Morphology and quantification of db/db and C57BL/6 islet extent. (A–C) Representative images taken of db/db and C57BL/6 islets using light microscopy in comparison: (A) typical small db islet with lost demarcation to exocrine issue, (B) example of extensive db islets, and (C) generic C57 islet (fuchsine red: insulin, bars indicate 50 µm). (D) Quantification of mean islet area as measured with ImageJ corresponding to islet extent. Black bars represent db/db mice, white bars represent C57BL/6 mice, n = 6 mice, * denotes p < 0.05.
3.3. Shift in Islet Cell Composition As a Sign of Uncontrolled Diabetes
In line with the diabetic phenotype images acquired for morphological studies also revealed faint insulin appearance in db/db when compared to the intense staining of C57BL/6 islets (Figures 3A–F). To further evaluate cell-specific pathologies, immunofluorescence staining of insulin and glucagon was conducted. This allowed for individual assessment of islet beta- and alpha-cell areas per islet and estimation of islet insulin and glucagon content from the same section.
Figure 3. Islet composition and insulin/glucagon content of db/db and C57BL/6 islets. (A–F) Representative images taken of immunostained db/db and C57BL/6 islets stained for insulin and glucagon (green: insulin, red: glucagon, bars indicate 50 µm). (G,H) Quantification of relative islet insulin and absolute glucagon area. (I) Quantification of islet glucagon/insulin area ratio. (J,K) Quantification of insulin and glucagon fluorescent intensity. Black bars represent db/db mice, white bars represent C57BL/6 mice, n = 6 mice, ** denotes p < 0.005, * denotes p < 0.05.
Analysis of immunostained slides indicated a shift in islet cell composition in db/db animals. Islets featured staining of alpha-cells in both the periphery and center with an overall increase in alpha-cell area as defined by positive staining of glucagon (Figures 3A–C). By contrast, C57 islets presented typical murine distribution patterns of peripheral alpha-cells (Figures 3D–F). Quantification of insulin and glucagon area per islet exposed a non-significant trend for higher absolute insulin area in non-diabetic wild-type mice (data not shown). However, relative insulin area normalized to islet extent demonstrated a significantly (p < 0.005) decreased value in db/db islets (Figure 3G). In contrast, absolute glucagon area in diabetic animals was significantly (p < 0.05) elevated (Figure 3H), while normalized glucagon area showed no significant difference between both strains of mice (data not shown). This shift in alpha- to beta-cell mass ratio in islets of diabetic mice was significant despite high variability in db/db islets (p < 0.005, Figure 3I).
Apart from this alteration of islet alpha- and beta-cell area, loss of staining intensity for insulin as well as glucagon was apparent. Quantitative analysis of fluorescent intensity was employed to assess islet insulin and glucagon content, confirming the optical impression of fainter staining in db/db islets with significantly lower fluorescent intensity for both proteins (p < 0.005 for insulin, p < 0.05 for glucagon, Figures 3J,K).
3.4. Distinct Grx5 Expression Patterns in Diabesity
In order to correlate the observed phenotypical and morphological differences between leptin-resistant, diabetic db/db animals and leptin-susceptible, non-diabetic controls with changes in expression of Grx5, we assessed islet Grx5 staining patterns in both strains of mice.
Both strains of mice featured global staining of islets cells with emphasis on nuclei as identified by comparing Grx5 and nucleus staining (Figures 4A–H). However, in db/db islets detection of Grx5-positive cells with nuclear staining was not as striking as in C57BL/6 islets. They exhibited a rather global and indistinct distribution of Grx5 with decreased intensity, and significantly (p < 0.005) lower Grx5-positive cell count. Quantification resulted in, on average, 25% Grx5-positive cells with nuclear staining in db/db islets and 49% in C57 islets (Figure 4L). In correspondence to generally enlarged islet size, diabetic mice were marked by significantly (p < 0.05) elevated Grx5 area (data not shown). When Grx5-positive cell area was normalized to islet extent this relation was reversed and a significant (p < 0.05) relative loss of Grx5 immunostaining was observed (Figure 4I). The differences in Grx5 expression between diabese and non-diabetic, lean controls could be further defined by quantification of Grx5 fluorescent intensity. Fluorescent intensity was significantly reduced in db/db islets, despite an increase in the area of positively stained cells, correlating with reduced islet Grx5 content (Figure 4J). The Grx5 to insulin content ratio was significantly (p < 0.0001) reduced in db/db islets (Figure 4K).
Figure 4. Grx5 expression patterns in db/db and C57BL/6 mice and quantification of Grx5 area, fluorescent intensity, Grx5 to insulin ratio and nuclei staining. (A–C,E–G) Representative images taken of immunostained db/db and C57BL/6 islets stained for insulin and Grx5 (green: insulin, red: Grx5, bars indicate 50 µm). (D,H) Schematics of Grx5 staining in db/db and C57BL/6 islets (black: high intensity staining to white: no signal detected). (I) Quantification of islet Grx5 area normalized to islet extent. (J) Quantification of Grx5 fluorescent intensity. (K) Quantification of Grx5 to insulin ratio. (L) Quantification of nuclei stained for Grx5. Black bars represent db/db mice, white bars represent C57BL/6 mice, n = 6 mice, *** denotes p < 0.0001, ** denotes p < 0.005, * denotes p < 0.05.
3.5. No Effect of Leptin on Grx5 Expression in Mouse Beta-Cells
Since the homozygous db mouse is an extreme example of total leptin resistance, our aim was to study whether leptin exposure to mouse beta-cells has influence on Grx expression. MIN6 cells were incubated with several concentrations of recombinant leptin for 2 and 48 h. As a control, MIN6 insulin content (Figure 5A) was measured in cell lysates and insulin secretion measured (Figure 5B) in supernatant. While insulin secretion declined significantly after 48 h of culture, no effect of leptin on insulin secretion was detected. Grx5 protein and mRNA expression were studied in MIN6 cells exposed to leptin. Grx5 protein expression featured a time-dependent non-significant increase toward 48 h which was independent of leptin concentration (Figure 5C). Grx5 mRNA expression decreased with time and was also not influenced by leptin (Figure 5D). Grx5 was not detected in cell supernatant (data not shown).
Figure 5. Insulin and Grx5 protein expression and Grx5 mRNA expression in MIN6 cells upon exposure to recombinant leptin for 2 and 48 h. (A) MIN6 lysate insulin content. (B) MIN6 supernatant insulin content. (C) MIN6 lysate Grx5 content. (D) MIN6 Grx5 mRNA expression. Black bars represent 2 h, white bars represent 48 h. n = 9 runs, *** denotes p < 0.001.
3.6. Beta-Cell Grx5 Expression Is Regulated by Hypoxia and Oleic Acid
Islet isolation of diabetic db/db mice presenting with uncontrolled diabesity for protein and mRNA analysis was not successful, due to the low yield of intact islets from db/db pancreases. Possible mechanisms behind deficiency of islet Grx5 content were, therefore, evaluated in vitro. MIN6 cells were exposed to oleic acid and hypoxia (2% O2) for 24 h. MIN6 secretion as measured by insulin content in cell supernatant was significantly attenuated under hypoxic treatment (p < 0.001). Exposure to oleic acid resulted in a non-significant trend of reduced insulin secretion (Figure 6A). Hypoxia significantly (p < 0.01) reduced INS2 mRNA expression, whereas treatment with oleic acid resulted in decreased expression; however, this was not significant (Figure 6B). Functional impairment of MIN6 cells upon hypoxic and oleic acid treatment was then correlated with Grx5 protein content and mRNA expression. In concordance with reduced insulin secretion and mRNA expression, MIN6 cells presented significantly reduced Grx5 protein content upon hypoxic (p < 0.01) and oleic acid (p < 0.05) incubation (Figure 6C). Both treatments attenuated Grx5 mRNA expression; however, effects were not significant (data not shown). To exclude beta-cell decay as a mediator for secretory impairment and reduction of Grx5, an MTT assay was conducted. MIN6 cells maintained strong viability upon exposure to oleic acid for 24 h under normoxia (Figure 6D).
Figure 6. Insulin and Grx5 protein and mRNA expression in MIN6 cells upon exposure to hypoxia (2% O2) and oleic acid for 24 h. (A) MIN6 supernatant insulin content. (B) MIN6 INS2 mRNA expression. (C) MIN6 lysate Grx5 content. (D) MIN6 MTT assay after 24 h of normoxic oleic acid treatment. Black bars represent normoxic atmosphere, white bars hypoxic atmosphere. n = minimum of 3 runs. *** denotes p < 0.001, ** denotes p < 0.01, * denotes p < 0.05.
4. Discussion
The glutaredoxin system has been repeatedly reported to exert protective effects on pancreatic beta-cells. In this study, we aimed to further elucidate these findings and evaluate a possible connection to histomorphological deviations of the islets of Langerhans occurring during uncontrolled diabesity as well as possible underlying mechanisms. Diabetic mice suffering from leptin-resistance on the db/db background were employed as a rodent model for diabetes mellitus type 2 and C57BL/6 wild-type animals without impairment of leptin signaling served as controls. As the utilized strain of db/db mice originates from a mixture of the C57BL/KsJ substrain and C57BL/6 wild-type mice (38, 39), they share a genetic background and thus provide a reasonable mouse model for our experimental setting.
A shift in islet cell composition associated with experimental diabetes is well documented (21, 22, 40, 41), but the underlying mechanisms are not fully understood. However, there is evidence that altered beta-cell functionality is profoundly involved in these histomorphological changes of the insulin-producing pancreatic micro organs. For instance, beta-cells were shown to express markers typically associated with endocrine progenitor cells in diabetes. Marked beta-cell plasticity was observed during progression of hyperglycemia as researchers reported beta-cell dedifferentiation into alpha-cells (23–25). Accordingly, beta-cells of hyperglycemic rodents including db/db mice feature loss of transcription factor Forkhead box protein O1 (FoxO1), an important regulator of beta-cell mass and stress response, which is accompanied by dedifferentiation into alpha-cells (23). Furthermore, levels of oxidative stress rise in pancreatic islets during diabetes (42). Oxidative stress is an acknowledged trigger of islet dysfunction (43) and maintenance of beta-cell differentiation is challenged by oxidative conditions (44). Islets of db/db mice typically present altered antioxidant enzyme expression, apart from Grxs (45), and modulation of oxidative stress markers (46) as well as increased ROS (33). Hypoxia has been described to occur in the beta-cells during high metabolic activity due to immensely high levels of oxidative phosphorylation (6, 7). As a result, a HIF-mediated hypoxic stress response is triggered (6) and apoptosis (6), upregulation of NF-κB, and oxidative stress (36) occur. Beta-cells are exceptionally vulnerable to hypoxia. In consequence, db/db islets present a marked increase in HIF and HIF target gene transcription (47) as well as NF-κB-mediated apoptosis (37). Free fatty acids have been reported to interfere significantly with beta-cell turnover (48) and induce functional and structural aberration of islets (49). These data indicate that the observed shift in islet cell composition is directly linked to impaired islet functionality mediated by gluco-/lipotoxicity and hypoxia. As a result, islets of db/db mice present pronounced structural deviations marked by a considerable amount of degranulated, i.e., endocrine inactive, beta-cells (50). Interestingly, Grxs are involved in regulation of oxidative stress, HIF (51) as well as NF-κB (52, 53). Beneficial effects of the Grx system on insulin secretion (54–56), as well as its impact on key enzymes of glucose metabolism (57–59), have been described. However, their role in pancreatic beta-cell function remains vague.
In the present histomorphological study, we identified distinct staining patterns of Grx5 with notable differences in expression between diabese mice and lean controls. Main features of Grx5 staining involved rarefication and loss of staining area as well as fluorescent intensity and Grx5 to insulin ratio in islets of diabetic mice. Strikingly, Grx5 presented a distinct staining of nuclei, which was mostly lost in diabetic islets. While Grx5 is an acknowledged mitochondrial glutaredoxin in yeast (14), it has been detected in rodent nuclei (8). However, the significance of this finding has yet to be elucidated. Grx5 is so far not known to exhibit catalytical activity, but Grx5-deficiency increases the susceptibility to oxidative stress (15) and correlates with cellular iron overload (17). These findings might account for Grx5 loss upon extensive metabolic stress; however, the observed loss of nucleic localization requires further study.
The homozygous db mice used in this study are hallmarked by complete leptin resistance (60) and thus exhibit a severe phenotype of diabesity (61). Adipokines and adipose-derived hormones are acknowledged mediators of inflammation, glucose and lipid metabolism, and energy balance (62). Leptin is an extensively studied hormone deriving from white adipose tissue (63). It is a key regulator of energy homeostasis (64) and exerts regulatory control on glucose metabolism and on the beta-cell itself in the so-called adipo-insular feedback loop. Leptin inhibits insulin secretion (65) and gene expression (66). In contrast, insulin increases leptin secretion (67) and gene expression (68). Expression of leptin correlates with fat mass leading to elevated levels in obese subjects (69, 70) as well as rodents (71). Homozygous db mice present complete leptin resistance. Therefore, influence of leptin excess on db/db islet Grx expression is highly unlikely. Our experimental setting was unable to deduce effects of leptin on insulin secretion or on Grx5 expression. In rodents, leptin plasma levels ranging from below 0.5 (72) up to 4,000 ng/ml (73) have been described. We deliberately chose leptin concentrations in a low physiological range to assess physiological influence on Grx5. Significant alterations of MIN6 insulin content and secretion occurred over time, as expected. While this poses a contradiction toward the adipo-insular axis, there are several differing reports in the current body of literature. Highly contingent on experimental settings and leptin dosage, studies reported no stimulation (74), stimulatory (75), and dose-dependent U-shaped responses in beta-cell lines, perfused pancreases, and isolated islets (76–78).
Interestingly, beta-cell Grx5 protein level correlated with insulin content. A non-significant decrease in Grx5 mRNA occurred over time, which we interpreted as a sign of sufficient Grx5 protein levels in beta-cells under physiological conditions in contrast to fading expression in islets of diabese animals. To elucidate a possible mechanism behind reduced Grx5 levels, MIN6 cells were exposed to hypoxia and oleic acid. Oleic acid as a monounsaturated fatty acid is typically elevated in the diabetic metabolism of db/db mice (79) and is a mediator of lipotoxicity. Concentrations characteristically occurring in diabetes (2, 80, 81) were used in beta-cell culture. Both stressors induced significantly attenuated Grx5 protein levels in MIN6 cells in correlation with reduced insulin secretion in vitro. Thus, Grx5 might be depleted in diabese rodents as part of the beta-cell’s extensive stress response to lipotoxicity and hypoxia. Especially as a mitochondrial protein, beta-cell and islet Grx5 content might further be reduced due to structural and functional deviations of mitochondria typically occurring in type 2 diabetes (82). Elevated mitochondrial ROS caused by lipotoxicity and hypoxia might be the link between mitochondrial damage and decreased levels of Grx5. Increased susceptibility to oxidative damage and impaired iron-homeostasis with iron-mediated ROS catalyzation as caused by Grx5-deficiency (15, 17) would even fuel this process.
Given our present data and little available literature, we can only speculate as to a connection between pronounced adjustment in Grx expression and islet remodeling under metabolic stress. Further studies are required, particularly functional in vivo experiments to gain deeper insights into the specific role of Grx5 for the islets of Langerhans. Glutaredoxin-regulated pathways involved in beta-cell physiology as well as targets and effectors of Grx need to be identified. No causal link between islet Grx expression and islet remodeling has been previously reported, but we have shown that it represents a promising target for future research. However, we were able to demonstrate clear qualitative and quantitative deviations in histomorphological glutaredoxin patterns in uncontrolled rodent diabesity when compared to lean wild-type controls and we were able to delineate the phenomenon from leptin resistance in vitro. Oleic acid and hypoxia were identified as possible mediators of beta-cell and islet Grx5-deficiency. The influence of further typical stressors present during diabesity on beta-cell Grx5 expression should be evaluated using a broader range of dosage. Results could hereafter be validated using a different rodent model. In addition, the direct link between hypoxic/lipotoxic stress and reduced islet Grx5 must be evaluated in vivo. The potential influence of HIF-dependent cell remodeling and gene transcription as source of altered endocrine beta-cell function should be ruled out.
In conclusion, we provide evidence for a connection between Grx5 expression and islet dysfunction during diabesity in vivo as well as a direct link between Grx5 and beta-cell insulin secretion which is independent from leptin resistance. In vitro culture of beta-cells under the influence of hypoxia and oleic acid reveals a potential mechanism of action. Our data support the role of Grx5 as a protective factor for the pancreatic beta-cell.
Ethics Statement
This study was carried out in accordance with the recommendations of institutional animal welfare officer, Chair of Animal Welfare of the Justus Liebig University Giessen, and Regional Administrative Council Giessen, Veterinary Department, under the code GI20/11-Nr.A18/2010. Both committees approved the protocol. All experiments were performed in accordance with German Animal Welfare Law. 3Rs were applied for reducing the number of required mice and reduce potential suffering, enrichment was applied to the IVC. Scoring for adverse events was done daily. Mice were anesthetized with isoflurane using a desiccator and sacrificed by cervical dislocation before removing the pancreas and other organs.
Author Contributions
Conceptualization: SFP and TL. Data curation, formal analysis, investigation: SFP, LMS, AK, and SR. Writing—original draft preparation: SP. Writing—review and editing: SFP, LMS, AK, SR, and TL. Guarantor of the research: TL.
Conflict of Interest Statement
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
Acknowledgments
TL is the guarantor of this work and, as such, had full access to all of the data in the study and takes responsibility for the integrity of the data and the accuracy of the data analysis. The authors thank Gundula Hertl, Birte Hussmann, and Doris Erb for expert advice and technical assistance. The authors thank Prof. Dr. Lillig, Department of Medical Biochemistry and Molecular Biology, Ernst-Moritz Arndt-University Greifswald, Germany, and Dr. Hanschmann, Department of Neurology, Heinrich Heine University Düsseldorf, Germany, for providing the antibody against Grx5. The authors thank Dr. Fiona Cousins for proofreading the manuscript.
Funding
This work was supported by Third Party Resources to TL from Clinical Research Unit and Justus Liebig University.
References
1. Robertson RP, Harmon J, Tran PO, Tanaka Y, Takahashi H. Glucose toxicity in beta-cells: type 2 diabetes, good radicals gone bad, and the glutathione connection. Diabetes (2003) 52(3):581–7. doi:10.2337/diabetes.52.3.581
2. Thiébaud D, DeFronzo RA, Jacot E, Golay A, Acheson K, Maeder E, et al. Effect of long chain triglyceride infusion on glucose metabolism in man. Metabolism (1982) 31(11):1128–36. doi:10.1016/0026-0495(82)90163-9
3. Solinas G, Naugler W, Galimi F, Lee M-S, Karin M. Saturated fatty acids inhibit induction of insulin gene transcription by JNK-mediated phosphorylation of insulin-receptor substrates. Proc Natl Acad Sci U S A (2006) 103(44):16454–9. doi:10.1073/pnas.0607626103
4. Cunha DA, Hekerman P, Ladrière L, Bazarra-Castro A, Ortis F, Wakeham MC, et al. Initiation and execution of lipotoxic ER stress in pancreatic beta-cells. J Cell Sci (2008) 121(Pt 14):2308–18. doi:10.1242/jcs.026062
5. Elsner M, Gehrmann W, Lenzen S. Peroxisome-generated hydrogen peroxide as important mediator of lipotoxicity in insulin-producing cells. Diabetes (2011) 60(1):200–8. doi:10.2337/db09-1401
6. Sato Y, Endo H, Okuyama H, Takeda T, Iwahashi H, Imagawa A, et al. Cellular hypoxia of pancreatic beta-cells due to high levels of oxygen consumption for insulin secretion in vitro. J Biol Chem (2011) 286(14):12524–32. doi:10.1074/jbc.M110.194738
7. Dionne KE, Colton CK, Yarmush ML. Effect of hypoxia on insulin secretion by isolated rat and canine islets of Langerhans. Diabetes (1993) 42(1):12–21. doi:10.2337/diabetes.42.1.12
8. Godoy JR, Funke M, Ackermann W, Haunhorst P, Oesteritz S, Capani F, et al. Redox atlas of the mouse. Immunohistochemical detection of glutaredoxin-, peroxiredoxin-, and thioredoxin-family proteins in various tissues of the laboratory mouse. Biochim Biophys Acta (2011) 1810(1):2–92. doi:10.1016/j.bbagen.2010.05.006
10. Chrestensen CA, Starke DW, Mieyal JJ. Acute cadmium exposure inactivates thioltransferase (Glutaredoxin), inhibits intracellular reduction of protein-glutathionyl-mixed disulfides, and initiates apoptosis. J Biol Chem (2000) 275(34):26556–65. doi:10.1074/jbc.M004097200
11. Gravina SA, Mieyal JJ. Thioltransferase is a specific glutathionyl mixed disulfide oxidoreductase. Biochemistry (1993) 32(13):3368–76. doi:10.1021/bi00064a021
12. Lill R, Dutkiewicz R, Freibert SA, Heidenreich T, Mascarenhas J, Netz DJ, et al. The role of mitochondria and the CIA machinery in the maturation of cytosolic and nuclear iron-sulfur proteins. Eur J Cell Biol (2015) 94(7–9):280–91. doi:10.1016/j.ejcb.2015.05.002
13. Stehling O, Wilbrecht C, Lill R. Mitochondrial iron-sulfur protein biogenesis and human disease. Biochimie (2014) 100:61–77. doi:10.1016/j.biochi.2014.01.010
14. Rodríguez-Manzaneque MT, Tamarit J, Bellí G, Ros J, Herrero E. Grx5 is a mitochondrial glutaredoxin required for the activity of iron/sulfur enzymes. Mol Biol Cell (2002) 13(4):1109–21. doi:10.1091/mbc.01-10-0517
15. Rodríguez-Manzaneque MT, Ros J, Cabiscol E, Sorribas A, Herrero E. Grx5 glutaredoxin plays a central role in protection against protein oxidative damage in Saccharomyces cerevisiae. Mol Cell Biol (1999) 19(12):8180–90. doi:10.1128/MCB.19.12.8180
16. Wingert RA, Galloway JL, Barut B, Foott H, Fraenkel P, Axe JL, et al. Deficiency of glutaredoxin 5 reveals Fe-S clusters are required for vertebrate haem synthesis. Nature (2005) 436(7053):1035–9. doi:10.1038/nature03887
17. Camaschella C, Campanella A, De Falco L, Boschetto L, Merlini R, Silvestri L, et al. The human counterpart of zebrafish shiraz shows sideroblastic-like microcytic anemia and iron overload. Blood (2007) 110(4):1353–8. doi:10.1182/blood-2007-02-072520
18. Baetens D, Malaisse-Lagae F, Perrelet A, Orci L. Endocrine pancreas: three-dimensional reconstruction shows two types of islets of Langerhans. Science (1979) 206(4424):1323–5. doi:10.1126/science.390711
19. Elayat AA, el Naggar MM, Tahir M. An immunocytochemical and morphometric study of the rat pancreatic islets. J Anat (1995) 186:629–37.
20. Steiner DJ, Kim A, Miller K, Hara M. Pancreatic islet plasticity: interspecies comparison of islet architecture and composition. Islets (2010) 2(3):135–45. doi:10.4161/isl.2.3.11815
21. McEvoy RC, Hegre OD. Morphometric quantitation of the pancreatic insulin-, glucagon-, and somatostatin-positive cell populations in normal and alloxan-diabetic rats. Diabetes (1977) 26(12):1140–6. doi:10.2337/diabetes.26.12.1140
22. Pipeleers D, in’t Veld PI, Maes E, Van De Winkel M. Glucose-induced insulin release depends on functional cooperation between islet cells. Proc Natl Acad Sci U S A (1982) 79(23):7322–5. doi:10.1073/pnas.79.23.7322
23. Talchai C, Xuan S, Lin HV, Sussel L, Accili D. Pancreatic beta cell dedifferentiation as a mechanism of diabetic beta cell failure. Cell (2012) 150(6):1223–34. doi:10.1016/j.cell.2012.07.029
24. White MG, Marshall HL, Rigby R, Huang GC, Amer A, Booth T, et al. Expression of mesenchymal and alpha-cell phenotypic markers in islet beta-cells in recently diagnosed diabetes. Diabetes Care (2013) 36(11):3818–20. doi:10.2337/dc13-0705
25. Gao T, McKenna B, Li C, Reichert M, Nguyen J, Singh T, et al. Pdx1 maintains beta cell identity and function by repressing an alpha cell program. Cell Metab (2014) 19(2):259–71. doi:10.1016/j.cmet.2013.12.002
26. Ebato C, Uchida T, Arakawa M, Komatsu M, Ueno T, Komiya K, et al. Autophagy is important in islet homeostasis and compensatory increase of beta cell mass in response to high-fat diet. Cell Metab (2008) 8(4):325–32. doi:10.1016/j.cmet.2008.08.009
27. Riahi Y, Wikstrom JD, Bachar-Wikstrom E, Polin N, Zucker H, Lee MS, et al. Autophagy is a major regulator of beta cell insulin homeostasis. Diabetologia (2016) 59(7):1480–91. doi:10.1007/s00125-016-3868-9
28. Unger RH, Aguilar-Parada E, Müller WA, Eisentraut AM. Studies of pancreatic alpha cell function in normal and diabetic subjects. J Clin Invest (1970) 49(4):837–48. doi:10.1172/JCI106297
29. Dusaulcy R, Handgraaf S, Heddad-Masson M, Visentin F, Vesin C, Reimann F, et al. alpha-cell dysfunctions and molecular alterations in male insulinopenic diabetic mice are not completely corrected by insulin. Endocrinology (2016) 157(2):536–47. doi:10.1210/en.2015-1725
30. Bloch K, Shichman E, Vorobeychik M, Bloch D, Vardi P. Catalase expression in pancreatic alpha cells of diabetic and non-diabetic mice. Histochem Cell Biol (2007) 127(2):227–32. doi:10.1007/s00418-006-0248-4
31. Hanschmann EM. Thioredoxin Family Proteins in Physiology and Disease [Dissertation] Marburg, Germany: Philipps-Universität Marburg (2011). doi:10.17192/z2011.0712
32. Stefanini M, De Martino C, Zamboni L. Fixation of ejaculated spermatozoa for electron microscopy. Nature (1967) 216:173–4. doi:10.1038/216173a0
33. Petry SF, Sharifpanah F, Sauer H, Linn T. Differential expression of islet glutaredoxin 1 and 5 with high reactive oxygen species production in a mouse model of diabesity. PLoS One (2017) 12(5):e0176267. doi:10.1371/journal.pone.0176267
34. Baltrusch S, Lenzen S. Novel insights into the regulation of the bound and diffusible glucokinase in MIN6 beta-cells. Diabetes (2007) 56(5):1305–15. doi:10.2337/db06-0894
35. Miyazaki J, Araki K, Yamato E, Ikegami H, Asano T, Shibasaki Y, et al. Establishment of a pancreatic beta cell line that retains glucose-inducible insulin secretion: special reference to expression of glucose transporter isoforms. Endocrinology (1990) 127(1):126–32. doi:10.1210/endo-127-1-126
36. Lai Y, Brandhorst H, Hossain H, Bierhaus A, Chen C, Bretzel RG, et al. Activation of NFkappaB dependent apoptotic pathway in pancreatic islet cells by hypoxia. Islets (2009) 1(1):19–25. doi:10.4161/isl.1.1.8530
37. Chen C, Moreno R, Samikannu B, Bretzel RG, Schmitz ML, Linn T. Improved intraportal islet transplantation outcome by systemic IKK-beta inhibition: NF-kappaB activity in pancreatic islets depends on oxygen availability. Am J Transplant (2011) 11(2):215–24. doi:10.1111/j.1600-6143.2010.03390.x
38. Hummel KP, Coleman DL, Lane PW. The influence of genetic background on expression of mutations at the diabetes locus in the mouse. I. C57BL-KsJ and C57BL-6J strains. Biochem Genet (1972) 7(1):1–13. doi:10.1007/BF00487005
39. Coleman DL. Obese and diabetes: two mutant genes causing diabetes-obesity syndromes in mice. Diabetologia (1978) 14(3):141–8. doi:10.1007/BF00429772
40. Cerf ME, Chapman CS, Louw J. High-fat programming of hyperglycemia, hyperinsulinemia, insulin resistance, hyperleptinemia, and altered islet architecture in 3-month-old Wistar rats. ISRN Endocrinol (2012):627270. doi:10.5402/2012/627270
41. Brereton MF, Iberl M, Shimomura K, Zhang Q, Adriaenssens AE, Proks P, et al. Reversible changes in pancreatic islet structure and function produced by elevated blood glucose. Nat Commun (2014) 22(5):4639. doi:10.1038/ncomms5639
42. Lenzen S. Chemistry and biology of reactive species with special reference to the antioxidative defence status in pancreatic beta-cells. Biochim Biophys Acta (2017) 1861(8):1929–42. doi:10.1016/j.bbagen.2017.05.013
43. Robertson RP. Chronic oxidative stress as a central mechanism for glucose toxicity in pancreatic islet beta cells in diabetes. J Biol Chem (2004) 279(41):42351–4. doi:10.1074/jbc.R400019200
44. Kondo T, El Khattabi I, Nishimura W, Laybutt DR, Geraldes P, Shah S, et al. p38 MAPK is a major regulator of MafA protein stability under oxidative stress. Mol Endocrinol (2009) 23(8):1281–90. doi:10.1210/me.2008-0482
45. Chan JY, Luzuriaga J, Bensellam M, Biden TJ, Laybutt DR. Failure of the adaptive unfolded protein response in islets of obese mice is linked with abnormalities in β-cell gene expression and progression to diabetes. Diabetes (2013) 62(5):1557–68. doi:10.2337/db12-0701
46. Lee Y-E, Kim J-W, Lee E-M, Ahn Y-B, Song K-H, Yoon K-H, et al. Chronic resveratrol treatment protects pancreatic islets against oxidative stress in db/db mice. PLoS One (2012) 7(11):e50412. doi:10.1371/journal.pone.0050412
47. Bensellam M, Maxwell EL, Chan JY, Luzuriaga J, West PK, Jonas JC, et al. Hypoxia reduces ER-to-Golgi protein trafficking and increases cell death by inhibiting the adaptive unfolded protein response in mouse beta cells. Diabetologia (2016) 59(7):1492–502. doi:10.1007/s00125-016-3947-y
48. Maedler K, Spinas GA, Dyntar D, Moritz W, Kaiser N, Donath MY. Distinct effects of saturated and monounsaturated fatty acids on beta-cell turnover and function. Diabetes (2001) 50(1):69–76. doi:10.2337/diabetes.50.1.69
49. Milburn J Jr, Hirose H, Lee YH, Nagasawa Y, Ogawa A, Ohneda M, et al. Pancreatic beta-cells in obesity. Evidence for induction of functional, morphologic, and metabolic abnormalities by increased long chain fatty acids. J Biol Chem (1995) 270(3):1295–9. doi:10.1074/jbc.270.3.1295
50. Leiter EH, Gapp DA, Eppig JJ, Coleman DL. Ultrastructural and morphometric studies of delta cells in pancreatic islets from C57BL/Ks diabetes mice. Diabetologia (1979) 17(5):297–309. doi:10.1007/BF01235886
51. Watanabe Y, Murdoch CE, Sano S, Ido Y, Bachschmid MM, Cohen RA, et al. Glutathione adducts induced by ischemia and deletion of glutaredoxin-1 stabilize hif-1α and improve limb revascularization. Proc Natl Acad Sci U S A (2016) 113(21):6011–6. doi:10.1073/pnas.1524198113
52. Hirota K, Matsui M, Murata M, Takashima Y, Cheng FS, Itoh T, et al. Nucleoredoxin, glutaredoxin, and thioredoxin differentially regulate NF-kappaB, AP-1, and CREB activation in HEK293 cells. Biochem Biophys Res Commun (2000) 274(1):177–82. doi:10.1006/bbrc.2000.3106
53. Daily D, Vlamis-Gardikas A, Offen D, Mittelman L, Melamed E, Holmgren A, et al. Glutaredoxin protects cerebellar granule neurons from dopamine-induced apoptosis by activating NF-kappa B via Ref-1. J Biol Chem (2001) 276(2):1335–44. doi:10.1074/jbc.M101400200
54. Reinbothe TM, Ivarsson R, Li DQ, Niazi O, Jing X, Zhang E, et al. Glutaredoxin-1 mediates NADPH-dependent stimulation of calcium-dependent insulin secretion. J Mol Endocrinol (2009) 23(6):893–900. doi:10.1210/me.2008-0306
55. Liu X, Han S, Yang Y, Kang J, Wu J. Glucose-induced glutathione reduction in mitochondria is involved in the first phase of pancreatic beta-cell insulin secretion. Biochem Biophys Res Commun (2015) 464(3):730–6. doi:10.1016/j.bbrc.2015.07.016
56. Takahashi HK, Santos LR, Roma LP, Duprez J, Broca C, Wojtusciszyn A, et al. Acute nutrient regulation of the mitochondrial glutathione redox state in pancreatic beta-cells. Biochem J (2014) 460(3):411–23. doi:10.1042/BJ20131361
57. Dong K, Wu M, Liu X, Huang Y, Zhang D, Wang Y, et al. Glutaredoxins concomitant with optimal ROS activate AMPK through S-glutathionylation to improve glucose metabolism in type 2 diabetes. Free Radic Biol Med (2016) 101:334–47. doi:10.1016/j.freeradbiomed.2016.10.007
58. Ward NE, Stewart JR, Ioannides CG, O’Brian CA. Oxidant-induced S-glutathiolation inactivates protein kinase C-alpha (PKC-alpha): a potential mechanism of PKC isozyme regulation. Biochemistry (2000) 39(33):10319–29. doi:10.1021/bi000781g
59. Wetzelberger K, Baba SP, Thirunavukkarasu M, Ho YS, Maulik N, Barski OA, et al. Postischemic deactivation of cardiac aldose reductase: role of glutathione S-transferase P and glutaredoxin in regeneration of reduced thiols from sulfenic acids. J Biol Chem (2010) 285(34):26135–48. doi:10.1074/jbc.M110.146423
60. Chen H, Charlat O, Tartaglia LA, Woolf EA, Weng X, Ellis SJ, et al. Evidence that the diabetes gene encodes the leptin receptor: identification of a mutation in the leptin receptor gene in db/db mice. Cell (1996) 84(3):491–5. doi:10.1016/S0092-8674(00)81294-5
61. Hummel KP, Dickie MM, Coleman DL. Diabetes, a new mutation in the mouse. Science (1966) 153(3740):1127–8. doi:10.1126/science.153.3740.1127
62. Flier JS, Cook KS, Usher P, Spiegelman BM. Severely impaired adipsin expression in genetic and acquired obesity. Science (1987) 237(4813):405–8. doi:10.1126/science.3299706
63. Zhang Y, Proenca R, Maffei M, Barone M, Leopold L, Friedman JM. Positional cloning of the mouse obese gene and its human homologue. Nature (1994) 372(6505):425–32. doi:10.1038/372425a0
64. Friedman JM, Halaas JL. Leptin and the regulation of body weight in mammals. Nature (1998) 395(6704):763–70. doi:10.1038/27376
65. Kulkarni RN, Wang ZL, Wang RM, Hurley JD, Smith DM, Ghatei MA, et al. Leptin rapidly suppresses insulin release from insulinoma cells, rat and human islets and, in vivo, in mice. J Clin Invest (1997) 100(11):2729–36. doi:10.1172/JCI119818
66. Seufert J, Kieffer TJ, Habener JF. Leptin inhibits insulin gene transcription and reverses hyperinsulinemia in leptin-deficient ob/ob mice. Proc Natl Acad Sci U S A (1999) 96(2):674–9. doi:10.1073/pnas.96.2.674
67. Laferrère B, Caixas A, Fried SK, Bashore C, Kim J, Pi-Sunyer FX. A pulse of insulin and dexamethasone stimulates serum leptin in fasting human subjects. Eur J Endocrinol (2002) 146(6):839–45. doi:10.1530/eje.0.1460839
68. Moreno-Aliaga MJ, Stanhope KL, Havel PJ. Transcriptional regulation of the leptin promoter by insulin-stimulated glucose metabolism in 3t3-l1 adipocytes. Biochem Biophys Res Commun (2001) 283(3):544–8. doi:10.1006/bbrc.2001.4822
69. Fain JN, Madan AK, Hiler ML, Cheema P, Bahouth SW. Comparison of the release of adipokines by adipose tissue, adipose tissue matrix, and adipocytes from visceral and subcutaneous abdominal adipose tissues of obese humans. Endocrinology (2004) 145(5):2273–82. doi:10.1210/en.2003-1336
70. Haleem DJ, Sheikh S, Fawad A, Haleem MA. Fasting leptin and glucose in normal weight, over weight and obese men and women diabetes patients with and without clinical depression. Metab Brain Dis (2017) 32(3):757–64. doi:10.1007/s11011-017-9964-9
71. Maffei M, Fei H, Lee GH, Dani C, Leroy P, Zhang Y, et al. Increased expression in adipocytes of ob RNA in mice with lesions of the hypothalamus and with mutations at the db locus. Proc Natl Acad Sci U S A (1995) 92(15):6957–60. doi:10.1073/pnas.92.15.6957
72. Hamad EM, Sato M, Uzu K, Yoshida T, Higashi S, Kawakami H, et al. Milk fermented by Lactobacillus gasseri sbt2055 influences adipocyte size via inhibition of dietary fat absorption in zucker rats. Br J Nutr (2009) 101(5):716–24. doi:10.1017/S0007114508043808
73. Singer G, Stokes KY, Terao S, Granger DN. Sepsis-induced intestinal microvascular and inflammatory responses in obese mice. Shock (2009) 31(3):275–9. doi:10.1097/SHK.0b013e3181834ab3
74. Leclercq-Meyer V, Malaisse WJ. Failure of human and mouse leptin to affect insulin, glucagon and somatostatin secretion by the perfused rat pancreas at physiological glucose concentration. Mol Cell Endocrinol (1998) 141(1–2):111–8. doi:10.1016/S0303-7207(98)00087-2
75. Tanizawa Y, Okuya S, Ishihara H, Asano T, Yada T, Oka Y. Direct stimulation of basal insulin secretion by physiological concentrations of leptin in pancreatic beta cells. Endocrinology (1997) 138(10):4513–6. doi:10.1210/endo.138.10.5576
76. Zhao AZ, Bornfeldt KE, Beavo JA. Leptin inhibits insulin secretion by activation of phosphodiesterase 3B. J Clin Invest (1998) 102(5):869–73. doi:10.1172/JCI3920
77. Brown JE, Dunmore SJ. Leptin decreases apoptosis and alters BCL-2: Bax ratio in clonal rodent pancreatic beta-cells. Diabetes Metab Res Rev (2007) 23(6):497–502. doi:10.1002/dmrr.726
78. Kieffer TJ, Heller RS, Leech CA, Holz GG, Habener JF. Leptin suppression of insulin secretion by the activation of ATP-sensitive K+ channels in pancreatic beta-cells. Diabetes (1997) 46(6):1087–93. doi:10.2337/diab.46.6.1087
79. Deepa SS, Walsh ME, Hamilton RT, Pulliam D, Shi Y, Hill S, et al. Rapamycin modulates markers of mitochondrial biogenesis and fatty acid oxidation in the adipose tissue of db/db mice. J Biochem Pharmacol Res (2013) 1(2):114–23.
80. Gordon E. Non-esterified fatty acids in blood of obese and lean subjects. Am J Clin Nutr (1960) 8(5):740–7. doi:10.1093/ajcn/8.5.740
81. Reaven GM, Hollenbeck C, Jeng CY, Wu MS, Chen YD. Measurement of plasma glucose, free fatty acid, lactate, and insulin for 24 h in patients with NIDDM. Diabetes (1988) 37(8):1020–4. doi:10.2337/diab.37.8.1020
Keywords: diabetes mellitus type 2, glutaredoxin, islet remodeling, rodent diabesity, db mouse, MIN6, lipotoxicity, hypoxia
Citation: Petry SF, Sun LM, Knapp A, Reinl S and Linn T (2018) Distinct Shift in Beta-Cell Glutaredoxin 5 Expression Is Mediated by Hypoxia and Lipotoxicity Both In Vivo and In Vitro. Front. Endocrinol. 9:84. doi: 10.3389/fendo.2018.00084
Received: 12 December 2017; Accepted: 22 February 2018;
Published: 12 March 2018
Edited by:
Åke Sjöholm, Gävle Hospital, SwedenReviewed by:
Toshiro Arai, Nippon Veterinary and Life Science University, JapanYukihiro Fujita, Asahikawa Medical University, Japan
Matteo A. Russo, IRCCS San Raffaele Pisana, Italy
Copyright: © 2018 Petry, Sun, Knapp, Reinl and Linn. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Sebastian Friedrich Petry, c2ViYXN0aWFuLnBldHJ5JiN4MDAwNDA7aW5uZXJlLm1lZC51bmktZ2llc3Nlbi5kZQ==