Metallothionein 1 negatively regulates glucose-stimulated insulin secretion and is differentially expressed in conditions of beta cell compensation and failure in mice and humans
The mechanisms responsible for beta cell compensation in obesity and for beta cell failure in type 2 diabetes are poorly defined. The mRNA levels of several metallothionein (MT) genes are upregulated in islets from individuals with type 2 diabetes, but their role in beta cells is not clear. Here we examined: (1) the temporal changes of islet Mt1 and Mt2 gene expression in mouse models of beta cell compensation and failure; and (2) the role of Mt1 and Mt2 in beta cell function and glucose homeostasis in mice.
Mt1 and Mt2 expression was assessed in islets from: (1) control lean (chow diet-fed) and diet-induced obese (high-fat diet-fed for 6 weeks) mice; (2) mouse models of diabetes (db/db mice) at 6 weeks old (prediabetes) and 16 weeks old (after diabetes onset) and age-matched db/+ (control) mice; and (3) obese non-diabetic ob/ob mice (16-week-old) and age-matched ob/+ (control) mice. MT1E, MT1X and MT2A expression was assessed in islets from humans with and without type 2 diabetes. Mt1-Mt2 double-knockout (KO) mice, transgenic mice overexpressing Mt1 under the control of its natural promoter (Tg-Mt1) and corresponding control mice were also studied. In MIN6 cells, MT1 and MT2 were inhibited by small interfering RNAs. mRNA levels were assessed by real-time RT-PCR, plasma insulin and islet MT levels by ELISA, glucose tolerance by i.p. glucose tolerance tests and overnight fasting-1 h refeeding tests, insulin tolerance by i.p. insulin tolerance tests, insulin secretion by RIA, cytosolic free Ca2+ concentration with Fura-2 leakage resistant (Fura-2 LR), cytosolic free Zn2+ concentration with Fluozin-3, and NAD(P)H by autofluorescence.
Mt1 and Mt2 mRNA levels were reduced in islets of murine models of beta cell compensation, whereas they were increased in diabetic db/db mice. In humans, MT1X mRNA levels were significantly upregulated in islets from individuals with type 2 diabetes in comparison with non-diabetic donors, while MT1E and MT2A mRNA levels were unchanged. Ex vivo, islet Mt1 and Mt2 mRNA and MT1 and MT2 protein levels were downregulated after culture with glucose at 10–30 mmol/l vs 2–5 mmol/l, in association with increased insulin secretion. In human islets, mRNA levels of MT1E, MT1X and MT2A were downregulated by stimulation with physiological and supraphysiological levels of glucose. In comparison with wild-type (WT) mice, Mt1-Mt2 double-KO mice displayed improved glucose tolerance in association with increased insulin levels and enhanced insulin release from isolated islets. In contrast, isolated islets from Tg-Mt1 mice displayed impaired glucose-stimulated insulin secretion (GSIS). In both Mt1-Mt2 double-KO and Tg-Mt1 models, the changes in GSIS occurred despite similar islet insulin content, rises in cytosolic free Ca2+ concentration and NAD(P)H levels, or intracellular Zn2+ concentration vs WT mice. In MIN6 cells, knockdown of MT1 but not MT2 potentiated GSIS, suggesting that Mt1 rather than Mt2 affects beta cell function.
These findings implicate Mt1 as a negative regulator of insulin secretion. The downregulation of Mt1 is associated with beta cell compensation in obesity, whereas increased Mt1 accompanies beta cell failure and type 2 diabetes.
KeywordsBeta cell compensation Beta cell failure Glucose-stimulated insulin secretion Islets Obesity Type 2 diabetes
Brown adipose tissue
Extensor digitorum longus
Carbonyl cyanide 4-(trifluoromethoxy)phenylhydrazone
- Fura-2 LR
Fura-2 leakage resistant
Glucose-stimulated insulin secretion
Small interfering RNA
Transgenic mice overexpressing Mt1 under the control of its natural promoter
White adipose tissue
Intracellular free Zn2+ levels
Type 2 diabetes results from the complex interplay of genetic and environmental risk factors, among which obesity plays a predominant role. Interestingly, most obese individuals compensate for insulin resistance by increasing insulin secretion, thereby maintaining normoglycaemia at the price of hyperinsulinaemia. However, this compensation can be sidestepped by a phase of decompensation in which beta cells fail to uphold an adequate secretory response [1, 2, 3]. This leads to hyperglycaemia and subsequent glucotoxic alterations of beta cell mass and function [4, 5]. Identifying genes involved in beta cell compensation in obesity, and in beta cell failure in type 2 diabetes may provide new insights into beta cell pathophysiology and reveal novel therapeutic targets to preserve beta cell function in individuals with (pre) type 2 diabetes.
Metallothioneins (MTs) are a family of low molecular mass, cysteine-rich, metal-binding proteins, the (patho)physiological functions of which have not been fully characterised. Their predominant roles are heavy metal detoxification, metal ion (including zinc) homeostasis, and the regulation of cellular redox status and antioxidant defences. Among the four different murine genes encoding MTs, Mt1 and Mt2 are expressed ubiquitously, Mt3 is mainly expressed in neurons and Mt4 is expressed in squamous epithelium cells. In humans, in addition to MT2 (also known as MT2A), MT3 and MT4, there are eight MT1 isoforms for a total of 11 functional MT genes [6, 7]. Interestingly, polymorphisms in MT1A and MT2A have been associated with increased risk for type 2 diabetes and diabetic complications [8, 9, 10]. Moreover, MT1E, MT1M, MT1X and MT2A mRNA levels were significantly upregulated in islets obtained by laser-capture microdissection (LCM) of pancreatic sections from type 2 diabetes donors . However, the role of MTs in the pathophysiology of type 2 diabetes remains unclear. We, therefore, verified whether changes in Mt1 and/or Mt2 gene expression plays a role in the modulation of beta cell function.
Fura-2 leakage resistant (Fura-2 LR), diazoxide (Dz), carbonyl cyanide 4-(trifluoromethoxy)phenylhydrazone (FCCP) and ZnCl2 were from Sigma (St Louis, MI, USA). N,N,N′,N′-tetrakis(2-pyridinylmethyl)-1,2-ethanediamine (TPEN) was from Abcam (Cambridge, UK). Fluozin-3, control non-targeting small interfering RNA (siRNA), ON-TARGETplus SMARTpool siRNA and DharmaFECT3 (transfection reagent) were from Thermo Fisher Scientific (Lafayette, CO, USA).
Six- and 16-week-old male and female C57BL/KsJ db/db mice and age-matched lean control mice (C57BL/KsJ), 16-week-old male and female C57BL/6J ob/ob mice and age-matched lean control mice, and the 16-week-old wild-type (WT) male mice (C57BL/6JAusb) used in diet-induced obesity experiments were from the Garvan Institute breeding colonies (Australian BioResources, Moss Vale, NSW, Australia). Male Mt1-Mt2 double-knockout (KO) mice at 4–5 months of age (129S7/SvEvBrd-Mt1tm1BriMt2tm1Bri/J; herein referred to as KO mice) and their sex- and age-matched controls (129S1/SvImJ) originated from the Jackson Laboratory (Bar Harbor, MA, USA). Male transgenic mice overexpressing Mt1 under the control of its natural promoter at 3 and 9 months of age (B6.Cg-Tg(Mt1)174Bri/J; referred to as Tg-Mt1) and their sex- and age-matched controls (C57BL/6 J) were also from the Jackson Laboratory. All animals were bred in the local animal facility of the health sciences sector at UCLouvain. Mice were housed under a controlled temperature of 22°C and a 12 h light cycle, with ad libitum access to water and chow (8% energy from fat, 21% energy from protein and 71% energy from carbohydrate [wt/wt]; 10.9 kJ/g; Gordon’s Specialty Stock Feeds, Yanderra, NSW, Australia) or a high-fat diet (HFD; 23% energy from fat, 19.4% energy from protein and 57.6% energy from carbohydrate and fibres [wt/wt for all]; 20.1 kJ/g; catalogue no. SF03-020; Specialty Feeds, Glen Forest, WA, Australia). Mice were randomly assigned to experimental groups using an odd/even number method by unblinded experimenters. All experiments were approved by the Institutional Committee on Animal Experimentation of the Health Sciences Sector at UCLouvain (Project 2013/UCL/MD/016) and the Garvan Institute/St Vincent’s Hospital Animal Experimentation Ethics Committee.
Human islets were obtained from 24 non-diabetic and 12 diabetic individuals at the Tom Mandel Islet Transplant Program, Melbourne . Human islets were isolated from heart-beating, brain-dead donors and approved for use under the ethics reference HREC011/04 (St Vincent’s Hospital Human Research Ethics Committee). Characteristics of donors and islet preparations are listed in the electronic supplementary material (ESM) Table 1. To evaluate the effects of glucose on MT gene expression, islets were obtained from three non-diabetic donors through the JDRF award 31-2008-416 (European Consortium for Islet Transplantation [ECIT] Islet for Basic Research program) and approved for use under the ethics reference B403/2017/05JUL/355 (Comité d’éthique hospitalo-facultaire Saint-Luc, UCLouvain). Characteristics of these donors are indicated in ESM Table 2. Written informed consent was obtained from next of kin and all experiments were performed in accordance with relevant guidelines and regulations.
Glucose and insulin tolerance tests
Intraperitoneal (i.p.) glucose tolerance tests (i.p.GTTs) and fasting-refeeding tests were performed on overnight-fasted mice and i.p. insulin tolerance tests (i.p.ITTs) on 4 h-fasted mice. For fasting-refeeding tests, blood glucose levels were measured in fasted mice and 1 h after refeeding. For i.p.GTTs and i.p.ITTs, mice were injected i.p. with glucose (2 g/kg of body weight) or insulin (0.75 U/kg of body weight; Actrapid, Novo Nordisk, Bagsværd, Denmark) and blood glucose levels were measured at the indicated time points using a FreeStyle Precision Neo glucometer (Abbott, Wavre, Belgium).
Tissue collection and histological analysis
Mice were killed by cervical dislocation and trunk blood collected and centrifuged for measurement of plasma insulin levels by ultra-sensitive ELISA (Crystal Chem, Downers Grove, IL, USA). The pancreas, liver, white adipose tissue (WAT) fat pads (epidydimal, retroperitoneal and inguinal), interscapular brown adipose tissue (BAT), skeletal muscles of the right leg (tibialis anterior, extensor digitorum longus [EDL], gastrocnemius and soleus) and heart of each animal were dissected, weighed, and frozen or fixed in 4% (wt/vol.) paraformaldehyde for 24 h at 4°C and embedded in paraffin for further histological analysis. Liver and epidydimal fat pad sections were counter stained with haematoxylin and eosin (H&E) to assess morphology. Adipocyte size was analysed using Visiopharm software (Author module, Version 6.4.1; Hørsholm, Denmark). Insulin and glucagon immunostaining of pancreatic sections was performed as previously described [13, 14]. Beta cell mass was computed based on the relative cross-sectional beta cell area and pancreas weight. Three pancreatic sections at three different levels were analysed for each mouse. Pancreatic sections immunoprobed for insulin, glucagon and a nuclear stain (DAPI) were scanned using the panoramic 250 Flash III digital slide scanner (3DHISTECH, Budapest, Hungary) and analysed with Visiopharm.
Islet isolation and culture
Islets were isolated by collagenase digestion, separated by density gradient centrifugation and handpicked under a stereomicroscope. Islets were cultured in standard RPMI medium (Invitrogen, Carlsbad, CA, USA) supplemented with 2 mmol/l glutamine, 5 g/l BSA, 100 U/ml penicillin and 100 μg/ml streptomycin.
Cell culture and treatment
MIN6 cells (passage 26–43; mycoplasma negative), originally provided by J. I. Miyazaki (Osaka University Medical School, Osaka, Japan) , were grown in Dulbecco’s modified Eagle’s medium (DMEM; Invitrogen) containing 25 mmol/l glucose, 10 mmol/l HEPES, 10% FCS (vol./vol.), 50 U/ml penicillin and 50 μg/ml streptomycin. Cells were transfected with 100 nmol/l control, Mt1 or Mt2 siRNA using DharmaFECT3 transfection reagent 24 h before experiments.
Glucose-stimulated insulin secretion (GSIS) tests
Isolated islets in batches of five, or MIN6 cells seeded in 24-well plates at 2 × 105 cell per well, were preincubated for 1 h in KRB buffer (120 mmol/l NaCl, 4.8 mmol/l KCl, 2.5 mmol/l CaCl2, 1.2 mmol/l MgCl2, 24 mmol/l NaHCO3 and 1 g/l BSA) containing 3 mmol/l glucose and then incubated for 1 h in KRB buffer containing 3 mmol/l, 15 mmol/l or 30 mmol/l glucose. At the end of the incubation, the buffer was collected for measurement of insulin by RIA, and islets were collected and disrupted by sonication in 10 mmol/l Tris, 0.2 mol/l NaCl and 10 mmol/l EDTA for measurement of their DNA and insulin content. All secretion experiments were carried out in duplicate.
NAD(P)H autofluorescence (excitation/emission wavelength [λex/em], 360/470 nm) was measured every 5 s and expressed as the percentage of the fluorescence level measured after 15–20 min of treatment with 10 μmol/l FCCP in KRB buffer containing 30 mmol/l glucose. For measurements of intracellular Ca2+ concentrations, islets were loaded for 2 h with 2 μmol/l Fura-2 LR acetoxymethyl ester and the fluorescence ratio (λex/em, 340/510 to 380/510 nm) was measured every 5 s. For measurements of intracellular free Zn2+ levels ([Zn2+]i), islets were loaded for 2 h with 2 μmol/l Fluozin-3 acetoxymethyl ester and fluorescence (λex/em, 490/510 nm) was measured every 10 s. TPEN (a zinc chelator) was used as a negative control to lower [Zn2+]i and used at 50 μmol/l. Islets from control and KO/Tg-Mt1 mice were simultaneously perifused side by side with KRB buffer continuously gassed with 5% CO2 air mix to maintain pH 7.4 at a flow rate of 1 ml/min at 37°C on the stage of an inverted microscope.
Total RNA was extracted and reverse transcribed as previously described [16, 17]. Real-time RT-PCR was performed using the SYBR Green method and a 7900HT Real-Time PCR System (Applied Biosystems, Foster City, CA, USA) or a CFX96 optical cycler detection system (Bio-Rad, Hercules, CA, USA). Primer sequences are listed in ESM Table 3. The value obtained for a specific gene product was normalised to the control gene cyclophilin A or TBP and expressed as fold change of the value in the control condition. TaqMan assays were used to assess the mRNA levels of MT1E (Hs01938284_g1), MT1X (Hs00745167_sH), MT2A (Hs02379661_g1) and the control gene 18S rRNA (Hs03003631_g1) in human islets from control and type 2 diabetes donors (Applied Biosystems). AmpliTaq Gold reagents (Thermo Fisher Scientific) were used on a Light Cycler 480 Instrument II (Roche, Risch-Rotkreuz, Switzerland).
Islet MT1 and MT2 protein levels were quantified by ELISA (Frontier Institute, Ishikari, Japan). Absorbance values were normalised to total protein content measured with the Pierce BCA Protein Assay Kit (Thermo Fisher Scientific).
Results are means ± SEM for the indicated number of experiments. Statistical significance was assessed by unpaired two-tailed Student’s t test, one-way ANOVA with a Newman–Keuls post hoc test, or two-way ANOVA with a Bonferroni post hoc test.
Mt1 and Mt2 mRNA levels were differentially regulated between conditions of beta cell compensation and failure
Glucose stimulation downregulated the expression of Mt1 and Mt2
MT1X mRNA levels were upregulated in human islets from individuals with type 2 diabetes and were affected by glucose stimulation
These results show that MT1X upregulation is associated with beta cell failure in human type 2 diabetes. They also reveal a specific gene expression pattern of human MT genes in response to glucose stimulation that partly resembles that of Mt1 and Mt2 in mouse islets.
Deletion of Mt1/Mt2 improved glucose tolerance
The potential role of Mt1 and/or Mt2 in the modulation of glucose homeostasis and beta cell function was investigated in a global Mt1-Mt2 double-KO mouse model . Compared with WT mice, KO mice displayed higher body weight and daily food intake (ESM Fig. 2a,b). They also showed increased liver weight (ESM Fig. 2c) without macroscopical or histological signs of steatosis (ESM Fig. 2d), and increased weight of different leg muscles, including tibialis anterior, EDL and gastrocnemius (ESM Fig. 2e–g). However, soleus muscle and heart weights were similar (ESM Fig. 2h,i). Interestingly, the weight of epidydimal, inguinal and retroperitoneal fat pads and the sum of the three fat pads (WAT), thereof, were reduced in KO mice (ESM Fig. 2j–m), whereas BAT weight was similar between KO and WT mice (ESM Fig. 2n). Histological sections of epidydimal fat pads also revealed reduced adipocyte surface in KO mice (ESM Fig. 2o,p).
MT deletion potentiated GSIS
We also measured the effects of acute stepwise increases in glucose concentration on intracellular NAD(P)H and Ca2+ levels and found no differences between WT and KO islets (Fig. 5g,h). These findings indicate that the potentiation of GSIS in KO islets results from an effect downstream of the stimulation of glucose metabolism and Ca2+ influx.
MTs are known for their metal-binding properties and proposed to play a role in metal ion, including zinc, homeostasis. As zinc plays a key role in beta cell biology, we used Fluozin-3 to compare the dynamic changes in [Zn2+]i in response to glucose and zinc supplementation/chelation in islets from WT and KO mice (ESM Fig. 3a). In islets from both mouse types, [Zn2+]i was increased upon supplementation of 3 mmol/l glucose-KRB buffer with 10 μmol/l ZnCl2, slightly decreased upon subsequent stimulation with 30 mmol/l in the continued presence of 10 μmol/l ZnCl2, rapidly decreased upon ensuing zinc chelation using TPEN, and markedly increased upon final addition of 1 mmol/l ZnCl2 to the medium. These effects were almost identical in WT and KO islets. In agreement, the mRNA levels of the key beta cell zinc transporters Zip6 (also known as Slc39a6), Zip7 (Slc39a7), Znt1 (Slc30a1) and Znt8 (Slc30a8) were similar between KO and WT islets (ESM Fig. 3b–e). These results rule out a potential role of changes in [Zn2+]i levels in the potentiation of GSIS in KO islets.
Assessment of the pancreas morphology revealed no difference in islet architecture between islets from WT and KO mice (ESM Fig. 4a). There were no significant changes in pancreatic weight, beta and alpha cell masses, or the percentage of alpha/beta cells per islet area between KO and WT mice (ESM Fig. 4b–e). Moreover, islets from WT and KO mice displayed no difference in the mRNA levels of the beta cell-enriched genes preproinsulin, Pdx1, Glut2 (also known as Slc2a2), Pcx and Gpd2 (ESM Fig. 4f–j). Similarly, there were no changes in the mRNA levels of the endoplasmic reticulum (ER) stress-response genes Hspa5 and Ddit3 (ESM Fig. 4k,l). Importantly, the deletion of Mt1 and Mt2 was not compensated for by upregulation of other MT genes. Thus, Mt3 mRNA levels were unchanged in islets from KO vs WT mice (ESM Fig. 4m), while Mt4 mRNA levels were undetected after 40 cycles of PCR amplification in both islet types.
Altogether, these findings strongly support a role for Mt1 as a negative modulator of GSIS.
Mt1 overexpression attenuated GSIS
Similarly, changes in [Zn2+]i in response to glucose and zinc supplementation/chelation were not different between islets from WT and Tg-Mt1 mice (ESM Fig. 6a). In agreement, the mRNA levels of zinc transporters Zip6, Zip7, Znt1 and Znt8 were unchanged in islets from Tg-Mt1 mice vs WT mice (ESM Fig. 6b–e).
Collectively, these findings further support the implication of Mt1 in the negative regulation of insulin secretion.
Overview of the principal findings of the study
Expression during beta cell compensation
Expression in T2D
Glucose effect on expression ex vivo
Effect of deletion/KD on GSIS
Effect of overexpression on GSIS
Mt1 and Mt2 exhibit an atypical gene expression pattern in comparison with other antioxidant genes
MTs are known for their protective antioxidant properties [26, 27, 28]. Oxidative stress plays an important role in beta cell demise and islets of humans with diabetes and animal models display upregulated expression of many antioxidant genes and markers of oxidative damage . Interestingly, antioxidant genes like Hmox1, Gpx1, Gpx2, Sod1 and Nrf2 (also known as Nfe2l2) were also upregulated in the islets of compensating young db/db mice and mice fed an HFD [17, 29, 30], in sharp contrast with Mt1 and Mt2 downregulation (Fig. 1). Similarly, in isolated islets, treatment with glucose upregulated Mt3, Srxn1 and Gpx2, while it downregulated Mt1 and Mt2 (Fig. 2 and [31, 32]). Noteworthy, our previous studies in Wistar rats revealed that islet Mt1 expression was upregulated by fasting and downregulated upon refeeding (J-C Jonas, unpublished data). Furthermore, a recent study exploring beta cell heterogeneity by single-cell transcriptomics revealed that high activity of the insulin gene promoter was associated with low expression of Mt1 and Mt2 and vice versa . These observations demonstrate that Mt1 and Mt2 behave differently from other oxidative stress-response genes. Besides, Mt1-Mt2 deletion does not affect antioxidant/stress-response gene expression (ESM Fig. 4 and ESM Fig. 7), indicating no evident impact on islet redox status under physiological conditions. Thus, Mt1 and/or Mt2 may play a role in beta cell (patho)physiology that goes beyond their known antioxidant function.
Mt1 negatively regulates GSIS
Deletion of Mt1 and Mt2 improved glucose tolerance and potentiated GSIS in isolated islets from KO mice. These findings contrast with a previous study using islets from Mt1-Mt2 KO mice . Although differences in genetic backgrounds may contribute to this discrepancy, our study is more comprehensive than the previous investigation. Thus, besides our complementary in vivo and ex vivo results, the knockdown of MT1 in MIN6 cells reproduced the enhanced insulin secretory phenotype of the KO islets. Furthermore, in our study, islets overexpressing Mt1 exhibited the reciprocal phenotype.
Our results underscore the role of Mt1, rather than Mt2, in the modulation of insulin secretion. Although these genes exhibit similar expression patterns, Mt1 displays a higher expression level in comparison with Mt2 and Mt3 in primary mouse islets (ESM Fig. 8). In addition, mRNA sequence alignment analysis showed that Mt1 and Mt2 are only ~80% identical. Thus, the ~20% sequence difference may also underlie functional specificities. Such specificities may stem from different metal affinities and binding properties or from specific protein–protein interactions [6, 35].
How could Mt1 impact on insulin secretion?
We did not detect significant changes in classical metabolic (NAD(P)H) and ionic parameters (cytosolic free Ca2+ and Zn2+) in response to glucose stimulation between islets from WT mice and KO or Tg-Mt1mice. The expression of antioxidant and other stress-response genes was not different between WT and KO islets, thereby ruling out a potential impact on redox status (ESM Fig. 4 and ESM Fig. 7). Furthermore, Mt1-Mt2 deletion or Mt1 overexpression had no impact on cell death in islets cultured under control conditions (10 mmol/l glucose; ESM Fig. 9). Nevertheless, insulin secretion in response to high potassium was also potentiated in islets from KO vs WT mice (ESM Fig. 10). This result strongly suggests a potential impact of Mt1 on the beta cell exocytotic machinery. Interestingly, MT3 was previously shown to interact with Rab3A GTPase in neurons, thereby playing a role in presynaptic vesicle trafficking . One may, therefore, hypothesise that MT1 interacts with a yet-to-be-identified protein of the beta cell exocytotic machinery to modulate insulin secretion.
The mechanism(s) of induction of Mt1 in diabetes
Hyperglycaemia, per se, may not be the upstream factor involved in increased expression of Mt1 in diabetes. Indeed, although Mt1 mRNA expression transiently increases in rat islets cultured overnight with glucose at 30 mmol/l vs 10 mmol/l , prolonged exposure of mouse and rat islets to high glucose (30 mmol/l) had little or no impact (vs 10 mmol/l) on Mt1 and Mt2 mRNA and MT1/MT2 protein levels (Fig. 2 and ). In human islets, culture in the presence of the already supraphysiological glucose concentration of 11.1 mmol/l vs 2.2 and 5.5 mmol/l also downregulated the mRNA levels of MT genes. Upregulation beyond this concentration may result from differences in glucose sensitivity and metabolism between human and mouse islets and may involve the activation of glucotoxicity-related pathways . We have previously shown that rat islet Mt1 expression is markedly induced by exogenous H2O2, the sarcoendoplasmic reticulum Ca2+-ATPase (SERCA) pump inhibitor thapsigargin, the cytokine IL-1β and hypoxia . However, the islet expression of genes induced by oxidative stress, ER stress and inflammatory stress are observed in the prediabetic stage in db/db mice , suggesting alternate mechanisms. On the other hand, evidence from several studies implicates a possible role of hypoxia: Mt1 mRNA expression is upregulated by hypoxia in mouse and human islets (ESM Fig. 11 and ), and a clear temporal in vivo association is observed between MT expression and an hypoxic gene expression signature in islets of db/db mice [39, 40].
Limitations of the study and perspectives
In this study, we used global KO animals. Since Mt1-Mt2 deletion may affect other metabolic tissues, one may argue that the observed secretory phenotype involves the effect of systemic factors. However, this is unlikely as we systematically precultured isolated islets for 1 week before GSIS tests. We also combined different models to demonstrate that Mt1 negatively regulates insulin secretion, i.e. by confirming the secretory phenotype after MT1 knockdown in MIN6 cells. Additionally, the attenuation of GSIS by Mt1 overexpression further supports our hypothesis. Although the Tg-Mt1 model is also global, it presents two important advantages: (1) the overexpression of the mouse Mt1 gene rather than human MT2A gene ; and (2) the control of Mt1 by its natural promoter rather than the insulin promoter, thereby avoiding the ER stress and oxidative stress observed in MT2A-transgenic mice . Indeed, our Tg-Mt1 islets displayed normal expression of ER stress-response genes (Fig. 8). Nevertheless, development of an Mt1-floxed mouse model is warranted for further exploration of these novel roles of Mt1 in beta cell biology.
Mt1 negatively regulates insulin secretion. Downregulation of islet Mt1 in obesity may, thus, contribute to beta cell compensation, and its upregulation in type 2 diabetes may contribute to beta cell failure. Inhibition of Mt1 may, therefore, represent an attractive therapeutic target to preserve and restore insulin secretion in type 2 diabetes.
We thank F. Knockaert (UCLouvain, Belgium) for expert technical help and J.-C. Henquin (UCLouvain, Belgium) for valuable discussion and suggestions. We also thank J. Duprez (UCLouvain, Belgium) for pilot experiments carried out in Mt-KO mice. Some of the data were presented as an abstract at the 54th EASD meeting in Berlin, Germany, 1–5 October 2018.
MB conceived the study and designed experiments, acquired and analysed most of the data and wrote the first draft of the manuscript. JCJ conceived the study and designed experiments, analysed data and revised the manuscript. YCS, JYC, DRL, HC, MAS, EGP and HET designed experiments, acquired and analysed data and critically reviewed the manuscript. PG contributed to the analysis and interpretation of the data and critically reviewed the manuscript. All authors approved the final version of the manuscript. MB is the guarantor of this work.
MB was supported by a MOVE-in Louvain/EC Marie-Curie incoming postdoctoral fellowship and is currently supported by a fellowship from the ‘Fonds de Recherche Clinique’, Cliniques Universitaires Saint-Luc, Brussels, Belgium. This work was supported by a grant from the Société Francophone du Diabète, Paris, France (SFD/MSD 2016), the Action de Recherche Concertée 12/17–047 from the Communauté française de Belgique, and the ‘Fonds Spécial de Recherche 2016’ from UCLouvain to JCJ. JCJ and PG are Research Directors of the Fonds de la Recherche Scientifique-FNRS, Belgium. JYC is supported by an NHMRC Early Career Fellowship. DRL is supported by an Australian Research Council (ARC) Future Fellowship. St Vincent’s Institute receives support from the Operational Infrastructure Support Scheme of the Government of Victoria.
Duality of interest
The authors declare that there is no duality of interest associated with this manuscript.
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