Consequences of Exposure to Light at Night on the Pancreatic Islet Circadian Clock and Function in Rats
- 1Larry L. Hillblom Islet Research Center, Department of Medicine, Division of Endocrinology, University of California, Los Angeles, David Geffen School of Medicine, Los Angeles, California
- 2Laboratory for Circadian and Sleep Medicine, Departments of Psychiatry and Biobehavioral Sciences, University of California, Los Angeles, David Geffen School of Medicine, Los Angeles, California.
- Corresponding author: Aleksey V. Matveyenko, .
There is a correlation between circadian disruption, type 2 diabetes mellitus (T2DM), and islet failure. However, the mechanisms underlying this association are largely unknown. Pancreatic islets express self-sustained circadian clocks essential for proper β-cell function and survival. We hypothesized that exposure to environmental conditions associated with disruption of circadian rhythms and susceptibility to T2DM in humans disrupts islet clock and β-cell function. To address this hypothesis, we validated the use of Per-1:LUC transgenic rats for continuous longitudinal assessment of islet circadian clock function ex vivo. Using this methodology, we subsequently examined effects of the continuous exposure to light at night (LL) on islet circadian clock and insulin secretion in vitro in rat islets. Our data show that changes in the light–dark cycle in vivo entrain the phase of islet clock transcriptional oscillations, whereas prolonged exposure (10 weeks) to LL disrupts islet circadian clock function through impairment in the amplitude, phase, and interislet synchrony of clock transcriptional oscillations. We also report that exposure to LL leads to diminished glucose-stimulated insulin secretion due to a decrease in insulin secretory pulse mass. Our studies identify potential mechanisms by which disturbances in circadian rhythms common to modern life can predispose to islet failure in T2DM.
Type 2 diabetes mellitus (T2DM) is characterized by islet failure due to loss of β-cell function and mass (1,2). The cause of islet failure in T2DM involves an interaction among genetic predisposition and confounding environmental factors (3). In recent years, environmental conditions associated with disruption of circadian rhythms (e.g., rotating shift work, light during the night, sleep loss, etc.) have become prevalent and have been reported to augment susceptibility to T2DM (4,5). Importantly, the correlation between circadian disruption and T2DM is partly attributed to loss of β-cell function and mass (6–8). Despite a strong association among circadian disruption, T2DM, and islet failure, the mechanisms underlying this link remain under investigation.
Circadian rhythms allow organisms to align internal metabolism as well as physiological and behavioral attributes to changes in the light–dark (LD) cycle. The “central clock” of the circadian system in mammals is localized in the suprachiasmatic nucleus (SCN) of the hypothalamus. The SCN consists of molecular oscillators (clocks), operating within individual neurons, governed by precise transcriptional-translational feedback loops (9). Moreover, molecular oscillators are also present in tissues outside of the SCN, including pancreatic islets (10). The SCN functions to synchronize peripheral clocks to the LD cycle via a combination of neuronal, behavioral, and endocrine outputs (11). The mechanism driving the molecular clocks is governed by a set of core “clock genes.” In short, CLOCK and BMAL1 are two helix-loop-helix transcription factors that are essential components of the core circadian clock (12), and when dimerized, activate transcription of the Period (PER) genes and Cryptochrome (CRY) genes through a circadian E-box regulatory element. Once translated, PER and CRY translocate to the nucleus where they function as negative regulators of their own transcription by interacting with the CLOCK/BMAL1 complex, thereby completing the negative feedback loop (13). This complex oscillatory network sustains 24-h transcriptional oscillations and, importantly, synchronizes transcription of clock effector genes to changes in the LD cycle (14).
Studies suggest that β-cell secretory function and survival is under transcriptional control of the circadian clock. β-Cell secretory capacity shows a circadian pattern, which is impaired upon exposure to aberrant LD cycles or SCN lesions (15–17). Circadian disruption in diabetes-prone rodents accelerates hyperglycemia through induction of islet failure (8). Moreover, clock gene mutants are hyperglycemic, glucose-intolerant, and lack appropriate insulin secretion (10,18,19). However, despite increased insights into the role of the circadian system in islet function, little data are available on the effects of environmental conditions associated with circadian disruption, common to modern life, on the integrity of the islet circadian clock and function. Consequently, to address this issue, we 1) validated the use of transgenic rats in which the Per-1 promoter was linked to a luciferase reporter (Per-1:LUC) for longitudinal assessment of islet circadian clock function ex vivo, 2) tested the hypothesis that changes in the LD cycle in vivo entrain the phase of islet clock transcriptional oscillations, and 3) tested the hypothesis that exposure to environmental conditions associated with circadian disruption (i.e., continuous exposure to light at night), disrupts islet circadian clock and function.
RESEARCH DESIGN AND METHODS
Animal husbandry and behavioral monitoring.
The study used 43 wild-type (WT) and 37 transgenic rats in which the mouse Period-1 promoter was linked to luciferase reporter (Per-1:LUC) rats. The generation and validation of Per-1:LUC rats has been previously described (20). Rats were housed individually at the University of California, Los Angeles (UCLA), animal facility and kept in environmentally controlled soundproof chambers under the standard 12/12-h LD cycle (lights on at 0600 h, lights off 1800 h, all times in Pacific Standard Time). Cages were outfitted with the optical beam sensor system to monitor circadian behavioral rhythms in activity and feeding (Respironics, Murrysville, PA). The UCLA Institutional Animal Care and Use Committee approved all experimental procedures.
Elucidation of behavioral, metabolic, and molecular circadian rhythms in WT rats under LD cycle.
To establish diurnal behavioral, metabolic, and temporal profiles in circadian clock gene and protein expression in vivo, we used 2-month-old WT rats. Rats were kept in the standard LD cycle for 10 weeks, and behavioral rhythms in feeding and activity were monitored. Rats were subsequently euthanized every 4 h (n = 4–5 per time point; at 0200, 0600, 1000, 1400, 1800, and 2200 h). Blood was immediately collected and the pancreas quickly excised, with one part preserved for immunohistochemical analysis and another for laser microdissection of islets for in vivo clock gene expression assessment by real-time PCR.
Laser microdissection of islets for assessment of profiles in islet clock gene expression in WT rats under LD cycle.
After euthanasia, the pancreas was harvested and embedded into optimal cutting temperature solution (Tissue-Tek, Torrance, CA), frozen on dry ice, and stored. Subsequently, complete longitudinal sections (8 μm) of pancreas were obtained using a precooled (−20ºC) cryotome and mounted on ultraviolet irradiated nucleic acid-free polyethylene naphthalate membrane slides (Leica, Wetzlar, Germany). Slides were then immediately stained with hematoxylin to identify islets and subsequently laser microdissected (Leica LMD7000) with ∼100 islets per time point per rat. Total islet RNA was isolated using Arcturus PicoPure extraction method (Applied Biosystems, Foster City, CA) and cDNA synthesis performed using the SuperScript III First-Strand synthesis kit (Invitrogen, Carlsbad, CA). The real-time PCR was performed with validated gene-specific primers for core clock genes (Bmal-1 and Per-1) according to the manufacturer’s instructions (7900HT Applied Biosystems).
Immunofluorescent staining for assessment of profiles in β-cell clock protein expression in WT rats under LD cycle.
After euthanasia, the pancreas was immediately harvested and fixed in 4% paraformaldehyde. Paraffin-embedded pancreatic sections were costained by immunofluorescence for markers of islet endocrine cell types insulin (18-0067; Invitrogen), glucagon (G2654, Sigma-Aldrich, St. Louis, MO), pancreatic polypeptide (NB100-1793, Novus Biologicals, Littleton, CO), somatostatin (MAB354, Millipore, Billerica, MA), and core clock proteins BMAL-1 (sc-8550), PER-1 (sc-25362), and PER-2 (sc-25363) obtained from Santa Cruz Biotechnology. Slides were viewed using a Leica DM6000 microscope (Leica Microsystems, Bannockburn, IL) and images acquired using OpenLab 5 (PerkinElmer, Waltham, MA).
Longitudinal assessment of rat islet circadian clock ex vivo using islets isolated from Per-1:LUC rats.
After euthanasia, rat islets were isolated from 2-month-old Per-1:LUC rats using standard collagenase method (performed always at 0900 Pacific Standard Time). Batches of 50 islets matched by size and diameter (using an ocular measuring device) were placed on PTFE membranes (Millipore) in culture dishes containing culture medium (serum-free, no sodium bicarbonate, no phenol red, Dulbecco’s modified Eagle’s medium [D50300-10L, Sigma-Aldrich] supplemented with 10 mmol/L HEPES [pH 7.2], 2 mmol/L glutamine, B27 [2%, GIBCO], and 0.1 mmol/L luciferin). To test glucose sensitivity of the islet clock (Fig. 2), culture medium was supplemented with 2, 5, 11, or 25 mmol/L d-glucose. For all subsequent studies (Figs. 3–6), islets were cultured in standard 11 mmol/L glucose rodent medium. Culture dishes containing islets were immediately placed into a LumiCycle luminometer (Actimetrics, Wilmette, IL) inside a light-resistant 37°C chamber with bioluminescence recorder photomultiplier tube detector. The bioluminescence signal was counted in 1-min bins every 10 min for at least 5 days, and data were normalized by subtraction of the 24-h running average from the raw data and then smoothed with a 2-h running average (Lumicycle Data Analysis, Actimetrics) (Supplementary Fig. 2). The peak was calculated as the highest point of smoothed data, and the free-running period was computed as the mean between the peaks in each cycle. The amplitude was summed by the highest point and the lowest point of the each cycle (21). Per-1–driven luciferase rhythms emanating from individual islets were imaged using an XR/MEGA-10Z cooled intensified charge-coupled device camera (Stanford Photonics, Inc., Palo Alto, CA). Isolated islets were cultured as previously described. Photon counts were integrated over 3 min with Piper control (Stanford Photonics) and processed with Image-J software (National Institutes of Health, Bethesda, MD). Amplitude, period, and the phase of Per-driven luciferase rhythms emanating from individual islets were calculated using Lumicycle Analysis software (Actimetrics). Phase coherence of islets was determined using Rayleigh plots, which were constructed by El-Temps software (Antoni Díez-Noguera, University of Barcelona, Barcelona, Spain).
Entrainment of the islet circadian clock by changes in the LD cycle.
To test whether changes in the LD cycle in vivo entrain the phase of islet clock transcriptional oscillations, we studied Per-1:LUC rats acclimatized for 2 weeks to the standard 12/12-h LD cycle. Behavioral recording was performed as described to confirm robust circadian behavioral rhythms. Subsequently, we inverted the phase of the LD cycle by 12 h to DL (lights on at 1800 h, lights off at 0600 h) for 4 weeks and confirmed entrainment to the new DL cycle using behavioral recordings. At the end of the 4-week period, DL rats were euthanized, islets isolated, and the amplitude, phase, and period of islet-specific Per-driven luciferase rhythms was determined as described.
Effects of circadian disruption due to light at night on behavioral, metabolic, and molecular circadian rhythms in WT rats.
Two-month-old WT rats were kept under lights on at night (LL) for 10 weeks, and induction of circadian arrhythmicity was confirmed by diurnal feeding and activity recordings. Subsequently, rats were euthanized every 4 h (n = 4–5 per time point; at 0200, 0600, 1000, 1400, 1800, and 2200 h) across the 24-h day, and blood and the pancreas were immediately collected for subsequent metabolic analysis.
We tested the hypothesis that chronic exposure to LL results in disruption of the islet clock function by studying nine Per-1:LUC rats. All rats were first acclimatized for 2 weeks to the standard LD cycle and then exposed to 10 weeks of the control LD cycle (n = 5) or 24-h LL (n = 4). Behavioral rhythms were monitored at baseline and during the study to confirm disruption of circadian rhythms in the LL rats. At the end of the 10-week experimental period, all LD and LL rats were euthanized, islets were isolated, and Per-1–driven bioluminescence rhythms were used to assess the amplitude, period, and the phase of the islet circadian clock, in batches of 50 islets (Fig. 4) and in individual islets (Fig. 5).
Islet isolations and assessment of β-cell function in vitro.
Pancreatic islets were isolated using standard collagenase procedure. To assess the dose-dependent glucose responsiveness, batches of 20 islets were statically incubated in RPMI solution supplemented with 4, 8, 12, and 16 mmol/L glucose for 30 min at each glucose concentration. Different batches of 20 islets were also stimulated with 10 nmol/L exendin-4 or 250 μmol/L tolbutamide for 30 min for assessment of non–glucose-dependent insulin release. Supernatant and lysed islets were assayed by insulin ELISA. To assess the pulsatile mode of insulin secretion, islet perifusion experiments were performed (ACUSYST-S, Cellex Biosciences, Inc., Minneapolis, MN) (22). Batches of 20 islets were first exposed to 40 min of 4 mmol/L glucose in Krebs-Ringer bicarbonate buffer supplemented with 0.2% serum albumin, preheated to 37ºC, and oxygenized with 95% O2 and 5% CO2, followed by 40 min of hyperglycemic perfusate (16 mmol/L glucose). Effluent was collected in 1-min intervals and assayed for insulin by ELISA for subsequent determination of total insulin secretory rate, insulin pulse mass, and insulin pulse interval (22).
Plasma glucose was measured by the glucose oxidase method (YSI Glucose Analyzer, Yellow Springs, OH). Insulin and C-peptide were measured using an ELISA assay (Alpco, Salem NH).
Statistical analysis and calculations.
Activity and feeding recordings were analyzed using ClockLab software (Actimetrics). Circadian rhythms in β-cell function and insulin sensitivity were calculated using homeostasis model assessment indices (HOMA) of insulin sensitivity (HOMAIR = [glucose] × [insulin]/405; insulin in mU/L and glucose in mg/dL) and β-cell function (HOMAβ = [20 × insulin]/[glucose − 3.5]; insulin in mU/L and glucose in mmol/L) (23). Statistical analysis was performed using ANOVA with the Fisher post hoc test where appropriate (Statistica; Statsoft, Tulsa, OK). Data in graphs are presented as means ± SEM and assumed statistically significant at P < 0.05.
Rats exhibit robust behavioral, metabolic, and molecular circadian rhythms under the LD cycle.
Noninvasive monitoring of locomotor activity and feeding was used to evaluate the integrity of the circadian system (24). As expected, WT rats kept in the standard LD cycle show robust 24-h behavioral rhythms (Fig. 1A and B). In addition, rats also display robust circadian rhythms in glycemia (peak: 2200 h, trough: 200 h, P < 0.05; Fig. 1C) and C-peptide secretion (peak: 2200 h, trough: 0600 h, P < 0.05; Fig. 1D). To assess islet clock gene expression in vivo, we performed laser microdissection of islets from pancreatic tissue sections collected during the 24-h LD cycle. Key circadian clock transcriptional activator Bmal-1 (peak: 0600 h, P < 0.05) and negative feedback regulator Per-1 (peak: 1800 h, P < 0.05) showed robust antiphase expression consistent with the proposed model of the mammalian circadian clockwork (Fig. 1E). Furthermore, immunofluorescence confirmed diurnal oscillations in clock protein expression localized to β-cells (Fig. 1F and Supplementary Fig. 1).
Longitudinal assessment of rat islet circadian clock using islets isolated from Per-1:LUC rats.
Tracking of cell bioluminescence with a clock gene luciferase fusion construct was used for assessment of islet circadian oscillators ex vivo (25). Islets cultured in standard islet media (11 mmol/L glucose) displayed sustained circadian rhythms in Per-1 bioluminescence, with a robust amplitude, oscillatory period, and the phase of circadian oscillations reflected the temporal profile of in vivo Per-1 mRNA expression (peak: 20.2 ± 0.6 h; Fig. 2A–D and Supplementary Fig. 2). Islet circadian clocks also demonstrated glucose sensitivity (Fig. 2A–D). Specifically, islets cultured at low glucose (2 or 5 mmol/L) showed a reduction in the amplitude (3.7-fold, P < 0.05 vs. 11 mmol/L), lengthening of the oscillatory period (27.5 ± 0.5 vs. 22.3 ± 0.1 h, P < 0.01 vs. 11 mmol/L), and altered phase (peak: 7 ± 0.9 vs. 20.2 ± 0.6 h, P < 0.05 vs. 11 mmol/L) of Per-1 bioluminescence oscillations (Fig. 2A–D). Exposure to hyperglycemic conditions (25 mmol/L) did not alter the amplitude, period, or the phase of the islet circadian clock (Fig. 2).
The amplitude of Per-1 bioluminescence in islets gradually dampened over time, as would be expected in the absence of the input from the SCN (21). However, activation of cAMP-response element binding protein (a mediator of circadian clock entrainment) with Forskolin (10 μmol/L) restarted Per-driven bioluminescence oscillations, confirming that dampening was not due to tissue attrition (Supplementary Fig. 3). Moreover, circadian oscillations in Per-1 bioluminescence were also detected from single islets that displayed robust in-phase oscillations (Fig. 2E and F).
Islet circadian clock is entrained by changes in the LD cycle.
We next investigated whether changes in the LD cycle can entrain and thus set the phase of islet clock transcriptional oscillations. To accomplish this, we inverted the phase of the LD cycle in Per-1:LUC transgenic rats by 12 h from LD (lights on at 0600 h, lights off at 1800 h) to DL (lights on at 1800 h, lights off 0600 h; Fig. 3A). Reversal of the LD cycle to the new DL cycle resulted in 12-h reversal of behavioral activity, confirming the success of the SCN photoentrainment (Fig. 3A and B). Subsequently, transition of the photoperiod from LD to DL resulted in near 12-h phase reversal of islet Per-1:LUC bioluminescence signal (peak: 22.2 ± 0.1 vs. 13.5 ± 0.6 h for LD vs. DL, P < 0.05; Fig. 3C and D) with no change in oscillatory period or the amplitude.
Circadian disruption due to LL disrupts islet circadian clock.
Increased exposure to LL disrupts circadian rhythms and augments susceptibility to T2DM in humans (26,27). Thus, we next set out to address whether chronic exposure to LL disrupts islet circadian clock function. We exposed 2-month-old Per-1:LUC rats to 10 weeks of the normal LD cycle or LL regimen. As expected, exposure to LL in rats resulted in behavioral arrhythmicity (Fig. 4A and B) and abolished circadian rhythms in calculated indices of insulin sensitivity and β-cell function derived from HOMA, HOMAIR, and HOMAβ (Fig. 4C and D). Importantly, exposure to LL led to the dampening in the amplitude of Per1-driven luciferase oscillations in isolated islets but did not affect the oscillatory period of Per1-driven oscillations (Fig. 4E and F). We further confirmed this observation at the single islet level by using intensified charge-coupled device camera recordings (Fig. 5). Whereas individual islets isolated from LD rats showed well-defined, in-phase, high-amplitude circadian cycles of Per1-driven luciferase expression, LL rats exhibited dampened amplitude (80%; LD vs. LL, P < 0.05; Fig. 5C) of circadian oscillations. Furthermore, Per-1 bioluminescence recorded from LL islets showed impaired phase and the synchrony of Per-driven luciferase oscillations among individual islets (peak: 22.5 ± 0.1 vs. 17.6 ± 0.5 h for LD vs. LL, P < 0.05; Fig. 5E). Interestingly, LL-treated islets still maintained a robust period of clock oscillations (Fig. 5D).
Effects of circadian disruption due to LL on β-cell function in vitro.
To assess whether prolonged exposure to LL has deleterious effects on β-cell secretory capacity, we exposed 2-month-old rats to 10 weeks of LD or LL cycle, confirmed disruption of circadian rhythms in LL via activity monitoring, and assessed insulin secretion in vitro in islets by static incubation and islet perifusion (Fig. 6). In islets isolated from LD animals, dose-dependent glucose stimulation induced by 8, 12, and 16 mmol/L glucose led to a robust increase in insulin release of approximately three-, four-, and fivefold versus 4 mmol/L, respectively (P < 0.05 at each glucose concentration; Fig. 6A and B). In contrast, LL islets showed blunted glucose-responsiveness, with only 16 mmol/L glucose eliciting a significant increase in insulin release from baseline (Fig. 6A and B). Insulin response to nonglucose secretory stimuli, such as exendin-4 and tolbutamide, remained intact in LL animals, suggesting a primary defect in glucose metabolism and/or coupling to oxidative phosphorylation (Fig. 6C). To elucidate the mechanism underlying diminished glucose-stimulated insulin release, we performed islet perifusions to assess the pulsatile mode of insulin secretion (Fig. 6D–I). LL-treated islets demonstrated blunted glucose-stimulated insulin secretion (∼40% vs. LD, P < 0.05), which was due to an ∼40% deficit in insulin secretory pulse mass, with no alteration in the frequency of pulsatile insulin release (Fig. 6D–I).
The mammalian circadian system is organized as a multilevel oscillator network. The main SCN oscillator is synchronized to the LD cycle through specialized retinal ganglion cells, with light serving as the principal entrainment stimuli (28). The SCN, in turn, plays a central role in synchronizing the rhythms of the peripheral circadian clocks to the 24-h LD cycle (29). This multilevel circadian oscillator system undoubtedly provides an evolutionary advantage for human health. However, because the circadian system is sensitive to changes in the LD cycle, disruption of circadian rhythms as a result of shift work, sleep loss, exposure to LL, and other factors has been associated with deleterious health consequences (30,31).
Specifically, circadian disruption is associated with development of T2DM, a relationship partly attributed to islet failure (5–8,10,18,19). This implicates disturbances in the islet circadian clock as a potential molecular mechanism underlying the association between circadian disruption, T2DM, and islet failure. Thus, in the current study, we sought to elucidate effects of the environmental conditions associated with circadian rhythm disruption common to modern life on the islet circadian clock and function. To address this, we first validated the use of Per-1:LUC rats for assessment of islet clock function ex vivo. Secondly, we established that changes in the LD cycles in vivo entrain the phase of islet clock transcriptional oscillations. Thirdly, we demonstrated that exposure to LL disrupts islet circadian clock function through impairment in the amplitude, phase, and interislet synchrony of clock transcriptional oscillations. Finally, we also report that islets isolated from rats exposed to LL exhibit diminished glucose-stimulated insulin secretion attributed to the deficit in insulin secretory pulse mass.
Evidence supports a role for the β-cell circadian clock in regulation of insulin secretion and β-cell survival. Circadian rhythms in glucose tolerance and β-cell secretory capacity have been observed under fasting, glucose-infusion, and meal conditions (15,32,33). Importantly, lesioning of the SCN in rats or exposure to LL abolishes circadian rhythms in glucose tolerance and insulin release and impairs β-cell function (16). This suggests that the central clock regulates diurnal insulin secretion, plausibly through influencing β-cell circadian clock function. In support of this hypothesis, pancreas-specific CLOCK and BMAL-1 mutant mice demonstrate a loss of diurnal rhythms in glucose tolerance and insulin secretion and exhibit diminished β-cell function (10,18). Furthermore, pancreas-specific clock mutants also show impaired expression of genes regulating islet growth, survival, and proliferation, emphasizing that the islet circadian clock may also be significant in the regulation of β-cell survival (10). Indeed, cellular response to oxidative and endoplasmic reticulum stress is under transcriptional control of the circadian clock (34). This is significant because both of these features contribute to islet failure in diabetes (35,36). Interestingly, circadian disruption due to prolonged exposure to LL in rats increases β-cell vulnerability to apoptosis associated with overexpression of human islet amyloid polypeptide, a known inducer of β-cell endoplasmic reticulum stress (8).
One of the key observations in our study is that exposure to LL leads to dampening, alterations in the phase, and desynchrony of islet clock transcriptional rhythms. This can be attributed to disruption or altered function of the SCN clock resulting in impaired entrainment of circadian oscillators in islets. Indeed, prolonged exposure to LL (of similar duration and light intensity used in our study) leads to desynchronization of circadian oscillators in the SCN, resulting in the loss of behavioral and endocrine rhythms (37). Similar abolishment of circadian behavioral and endocrine rhythms is observed after SCN lesioning in rodents, which can be partially restored upon SCN transplantation (38,39). Importantly, SCN lesions are associated with damping of the amplitude of circadian clock oscillations in peripheral tissues (e.g., liver and kidney) (40,41), albeit with some studies only noting alterations in the phase of transcriptional oscillations (42). Consistent with our findings, these studies suggest that surgical or light-induced disruption of the SCN circadian clock can result in impaired cyclical expression, dampened amplitude, and altered phase of circadian clock transcriptional oscillations in peripheral tissue. Moreover, our work also shows that in some parallels to the results obtained by lesioning the SCN (37), exposure to LL results in impaired coupling among individual circadian oscillators in pancreatic islets. The functional significance of uncoupling individual circadian oscillators in islets is unknown; however, synchronization of individual neuronal clocks in the SCN is essential for proper clock function (43).
Mechanisms have been proposed to mediate entrainment of peripheral oscillators by the SCN (29). However, which mechanism(s) regulate entrainment of islet circadian clocks are currently unknown. The SCN has been shown to modulate peripheral clock expression through the autonomic nervous system (44). Pancreatic islets receive extensive innervation by the autonomic nervous system, and the SCN has been shown to innervate the pancreas via the parasympathetic neuronal pathway (45). The SCN also has been shown to modulate entrainment of peripheral clocks through circadian regulation of hormonal release (e.g., corticosterone and melatonin) (29). Recent work on the role of melatonin receptor signaling in the regulation of islet failure in T2DM suggests that the significance of diurnal melatonin secretion for entrainment of islet clocks merits further investigation (46). In addition, the SCN also controls diurnal feeding, the timing of which has been shown to entrain the phase and the amplitude of peripheral clocks, particularly in organs, such the liver and the pancreas, responsive to nutrient availability (20,47). In our study, exposure to LL was associated with the loss of circadian rhythms in hormonal release (melatonin and corticosterone) and in feeding behavior. However, further work is needed to delineate exact mechanisms regulating entrainment of clocks in islets.
This report also examined effects of prolonged exposure to LL on β-cell function in isolated islets. Our observation that prior exposure to LL results in diminished β-cell function is consistent with findings in humans that report induction of glucose intolerance and diminished insulin response to glucose after circadian misalignment (7,17). Our data are also consistent with findings reported in rodents with genetic mutations in the core components of the circadian clock genes, which also demonstrate diminished β-cell glucose-responsiveness hypothesized to be associated with defective insulin exocytosis and/or mitochondrial uncoupling leading to diminished glucose-induced mitochondrial potential and ATP production (10,48).
In conclusion, we established and validated methods for continuous longitudinal monitoring of islet circadian clocks ex vivo using Per-1:LUC rats. Using this methodology, we demonstrated that islet clock transcriptional oscillations are entrained by changes in the LD cycle and found that disruption of circadian rhythms due to exposure to LL disturbs islet circadian clock and β-cell function in vitro. Our data suggest that impaired islet clock function caused by circadian system disruption may be responsible for altered islet function and survival and consequent predisposition to T2DM.
This work was supported by grants from the National Institutes of Health (K01DK089003) and the Larry L. Hillblom Foundation to A.V.M. and the Esther B. O’Keefe Foundation to A.V.M. and C.S.C.
No potential conflicts of interest relevant to this article were reported.
J.Q. assisted with design of the studies, performed studies, and assisted with interpretation of the studies and preparation of the manuscript. G.D.B. and C.S.C. assisted with study design and interpretation and reviewed and edited the manuscript. A.V.M. contributed to study design and interpretation and wrote the manuscript. A.V.M 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 the members of the laboratories of Dr. Joseph Bass (Northwestern University) and Dr. Christopher Colwell (UCLA) for excellent suggestions in developing conditions for islet bioluminescence recordings. The authors are grateful to Bonnie Yeh (UCLA) and Kevin Hsu (UCLA) for excellent technical support and animal care. The authors also thank Dr. Peter C. Butler (UCLA) for helpful discussions and insightful comments.
This article contains Supplementary Data online at http://diabetes.diabetesjournals.org/lookup/suppl/doi:10.2337/db12-1543/-/DC1.
- Received November 6, 2012.
- Accepted June 11, 2013.
- © 2013 by the American Diabetes Association.
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