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Department of Biomedical Sciences, Atlantic Veterinary College, University of Prince Edward Island, 550 University Avenue, Charlottetown, Prince Edward, C1A 4P3 Canada
1 Departments of Medicine and Physiology, University of Toronto, 1 Kings College Circle, Toronto, Ontario, M5F 1A8 Canada
(Requests for offprints should be addressed to C B Chan; Email: cchan{at}upei.ca)
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Abstract |
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Introduction |
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The enzyme adenylate cyclase catalyzes the conversion of ATP to cAMP, an important second messenger involved in potentiating rather than initiating insulin secretion (Prentki & Matschinsky 1987). Deficient cAMP production has been implicated in streptozotocin diabetes (Dachicourt et al. 1996), while increasing cAMP with forskolin improved GSIS in Goto-Kakizaki (GK) rats (Abdel-Halim et al. 1996). It is unknown whether enhancing cAMP production can ameliorate insulin secretion in ob/ob mice or other models where UCP2 is upregulated.
cAMP is proposed to influence insulin secretion at multiple steps via two distinct pathways, one mediated by protein kinase A (PKA) and the other by cAMP-regulated guanine nucleotide exchange factors (cAMP-GEFs, also known as epac; Holz 2004). Two important cAMP-dependent steps that also require adequate intracellular ATP are exocytosis, including regulation and replenishment of the readily releasable pool of granules (Kashima et al. 2001, Eliasson et al. 2003) and ATP-dependent potassium (KATP) channel inactivation (MacDonald et al. 2002).
We tested the hypothesis that elevation of cAMP subsequent to upregulation of UCP2 expression will normalize insulin secretion because cAMP is an important potentiator of GSIS, acts at many steps in stimulus-secretion pathways of ß-cells and has been shown to ameliorate defective insulin secretion in other models.
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Materials and Methods |
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All animals used in the present research were cared for in accordance with the Guidelines of the Canadian Council on Animal Care. The protocols were approved by animal use committees from the University of Toronto and the University of Prince Edward Island. Rats were anesthetized with sodium pentobarbital (0.1 ml/100 g). Islets were harvested from 10-week-old male and female lean Zucker rats (Charles River Laboratories, Boston, MA, USA and AVC born) and from 8-week-old lean and ob/ob mice (Jackson Labs, Bar Harbour, ME) and cultured as described (Kibenge & Chan 1995).
Adenoviral infection of rodent islets
Islets were infected with adenovirus encoding the full-length human or rat cDNA for ucp2 (Aducp2) as described (Chan et al. 1999, 2001, Joseph et al. 2004) for 48 h. Control islets received no treatment and were simply cultured in DMEM (Ducbecco’s modified Eagle medium; Invitrogen) for 48 h, because non-specific adenoviral infection had not been shown to affect insulin secretion (Chan et al. 1999). In some experiments, isolated rat islets were cultured overnight in DMEM supplemented with 10 µM forskolin (Sigma). Over-expression of ucp2 was confirmed by quantitative reverse transcriptase (RT)-PCR as described (Joseph et al. 2002).
Perfused mouse pancreas
Control (wild type, WT) and ucp2 knockout (KO) mice were raised in a colony at the University of Toronto. Generation of the KO line has been described previously (Zhang et al. 2001). The pancreases from 4-month-old male ucp2 KO mice were perfused after an overnight fast. The anesthetic was i.p. sodium pentobarbital (80 mg/kg). Details of the perfusion protocol are given elsewhere (Joseph et al. 2002). In these experiments, the glucose infusion was changed from 1.4 to 13.4 mM after 5 min, then returned to 1.4 mM at 25 min. Exendin-4 (1 nM, Bachem, Bubendorf, Switzerland), which acts as an agonist at GLP-1 receptors (Raufman et al. 1992) was added in some experiments.
Cell culture and transient transfection of ßTC-6f7 cells
Cultures of ßTC-6f7 (ß-TC) cells were grown in RPMI-1640 media (Invitrogen), pH 7.4 as described (Chan et al. 2001). For transient gene transfection, ß-TC cells were plated at a density of 2.5 x 105 cells/cm2 and cultured overnight. Plasmids containing either ucp2 or enhanced green fluorescent protein (egfp) cDNA were produced as described (Chan et al. 2001) and transfection carried out as per the instructions of the manufacturers of the transfection agent (Lipofectamine2000, Invitrogen). The degree of ucp2 overexpression (ucp2-OE) induced was assessed by quantitative RT-PCR, as for rat islets (Joseph et al. 2002).
cAMP content
Control and ucp2-OE islets were exposed to 0–10 µM forskolin (Sigma) or exendin-4 (1 nM) in the presence of 2.8 or 11 mM glucose in KRBB–HEPES for 15 min at 37 °C. The medium was then removed and 70% ethanol (0.5 ml/well) was added to the cell pellets. Cell lysates were frozen at –20 °C until assayed by RIA using the acetylation protocol provided in the kit for increased sensitivity (Biomedical Technologies, Inc., Stoughton, MA, USA).
Insulin secretion from cell lines or islets
Control and ucp2-OE ß-TC cells or islets were prepared as described for cAMP formation and incubated for 2 h at 37 °C. Where indicated in the Results, additional test compounds were added to islet incubations. The PKA inhibitors, H89 and KT5720 (Sigma), were added to test wells 30 min prior to the addition of forskolin for a further 90 min. The medium was aspirated and placed in clean 1.5 ml microcentrifuge tubes, which were then centrifuged briefly to remove cellular debris. To each cell pellet, 1 ml 3% acetic acid was added to extract the total remaining insulin. All samples were frozen at –20 °C until assayed. Concentrations of insulin were determined by RIA.
Protein kinase A activity
The effects of ucp2-OE on PKA activity were assessed in rat islets using a colorimetric assay (Stressgen, Victoria, BC, Canada). Control and ucp2-OE islets (100 per condition) were incubated with 1 µM forskolin ± 10 µM H89 (Calbiochem, La Jolla, CA, USA) for 30 min, and washed in 0.5 ml PBS (pH 7.4). The islet cytosol was reserved following the cell lysis as recommended in the manufacturer’s instructions. The lysate (60 islet equivalents in 30 µl aliquots) was incubated for 30 min with the ATP substrate. Detection of phosphorylated proteins was facilitated by incubation with phosphoprotein-specific antibody. Although the assay was performed with crude extracts, the ability to inhibit most of the activity with H89 suggests that the majority of kinase activity was due to PKA.
ATP content
ATP and ADP were quantified in ucp2 KO mouse islets by the method of Schultz et al.(1993).
Assessment of KATP channel activity
Efflux of radiolabeled 86Rb+ was quantified to estimate changes in K+channel activity in islets as described previously (Chan & MacPhail 1996). Islets were loaded with 86RbCl (Amersham) for 90 min at 37 °C, during which time the radiolabel was taken up into the islet cells. After washing twice, the islets were resuspended in KRBB–HEPES containing low (2.8 mM) or high (11 mM) glucose to determine what degree of K channel activity was glucose metabolism-dependent and therefore reflective of KATP channels. In some tubes, 1 µM forskolin ± 1 µM H89 were also added. After 20 min, the supernatant buffer and the islet pellets were transferred to clean vials for scintillation counting. Results were expressed as the fractional efflux of 86Rb+/20 min.
Electrophysiological assessment of KATP channel activity was performed using patch clamping of intact islets infected with control (AdEmpty) or Aducp2 virus. Islets were held in the recording chamber with the assistance of a suction pipette. KATP current was measured in the perforated-patch configuration during 200 ms 20 mV incremental step-depolarizations from –140 to –60 mV from a holding potential of –70 mV. Mean outward current at each potential was measured during the last 50 ms of depolarization. The pipette solution contained (mM) K2SO4 28.4, KCl 63.7, NaCl 11.8, MgCl2 1, HEPES 20.8, EGTA 0.5, pH 7.2 with KOH+0.1 mg/ml amphotericin B (Sigma). The bath solution contained (mM) NaCl 115, CaCl2 3, KCl 5, MgCl2 2, glucose 11.1, HEPES 10, pH 7.2 with NaOH. Islets were held in a static bath maintained at 34 °C by an automatic temperature controller (TC-324B, Warner Instrument Corp., Hamden, CT, USA). Current recordings were amplified, digitized, and analyzed using pClamp9.0 software (Axopatch 200B, Axon Instruments, Union City, CA, USA).
Calcium flux measurement
ß-TC cells or ß-cells from dispersed islets were plated on glass coverslips (about 80% confluency) and transfected with plasmid encoding ucp2 or egfp (control) as described in Chan et al.(2001). Fluorescent measurements were conducted 48 h after transfection. Changes in intracellular Ca2+ concentrations were assessed using Fura 2-AM. The cells were loaded with 5 µM Fura 2-AM for 50 min in a medium containing (in millimolar) 130 NaCl, 5 KCl, 2 CaCl2, 1 MgCl2, 5 NaHCO3, 10 HEPES, pH 7.4 at 37 °C. The cells were then washed, transferred to an open chamber, placed on an Olympus BX51W1 fluorescent microscope stage and perfused with the same medium at 1 ml/min. All experiments were performed at 36–37 °C using a TC-324B Heater Controller (Warner Instruments). For excitation, a xenon lamp-based DeltaRam high-speed monochromator (Photon Technology International, London, ON, Canada) was used. Cells were excited by dual excitation at 340/380 nm and emission was detected by a 510 nm band pass filter. For control of the monochromator and videocamera, as well as for fluorescent imaging and collecting of data the ImageMaster 3 software (Photon Technology International) was used. The basal intracellular Ca2+concentration ([Ca2+]i) was calculated according to the equation [Ca2+]i = Kd x ß x (R–Rmin)/(R–Rmax), where R is the fluorescence ratio at 340 and 380 nm excitations (F340/F380), Rmin and Rmax are the fluorescence ratios at Ca2+- free and Ca2+-saturating conditions, Kd is the dissociation constant ( = 224 nM), and ß = F380 (Ca2+-free)/F380 (Ca2+-saturating). Saturating and Ca2+-free conditions were obtained by the addition of 10 µM ionomycin (Sigma) to cells incubated with 5 mM Ca2+, and by addition of 10 mM EGTA to cells incubated in Ca2+-free medium.
Statistical analysis
Data are presented as means ± S.E.M. Results were compared by unpaired t-test, one- or two-way ANOVA, where applicable, and P < 0.05 was considered significant. Prism 3.0 software (GraphPad, San Diego, CA, USA) was used for the statistical analysis.
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Results |
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To determine if forskolin could restore GSIS in a model of insulin insufficiency and documented overexpression of UCP2 (Zhang et al. 2001), islets were obtained from lean and ob/ob mice. In these experiments, ob/ob islets had a ~twofold increase in ucp2 mRNA expression compared with age-matched lean mouse islets (Table 1
). In lean islets, glucose alone increased insulin secretion by ~twofold over basal. Forskolin potentiated the response to higher glucose concentrations (Fig. 1A). Basal insulin secretion was elevated in ob/ob mice and there was no response to glucose. Addition of 10 µM forskolin significantly increased the insulin secretion at glucose concentrations from 5.5 to 22.0 mM (Fig. 1B).
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Infection of rat islets with Aducp2 induced an 19-fold increase in ucp2 mRNA (Table 1
). In these experiments, the ability of forskolin, an adenylate cyclase activator, to stimulate insulin secretion was tested. Both UCP2 expression (P < 0.0001) and forskolin concentration (P < 0.0001) influenced insulin secretion. A significant two-way interaction (P < 0.005) revealed that ucp2-OE cells responded differently compared with control islets to forskolin. Insulin secretion from Aducp2-infected cells was lower than control cells at 0 and 0.1 µM forskolin (P < 0.03) but was not different at 1 and 10 µM forskolin (Fig. 2A). Thus, at higher doses, forskolin normalized insulin secretion in Aducp2-infected rat islets. Similar effects were observed in clonal ß-TC cells (not shown; Chan et al. 2001).
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shows that inhibition of PKA by H89 and KT5720 blocked the stimulatory effects of forskolin on insulin secretion in both ucp2-OE and control islets. That ucp2-OE had no effect on PKA activity in islets is verified in Fig. 2C. Moreover, the increase in PKA activity, as measured by the production of phosphoproteins, was totally negated in the presence of 10 µM H89. cAMP concentrations were measured following exposure to forskolin in rat islets that had normal or elevated ucp2 mRNA expression. In the presence of 11 mM glucose, a similar concentration response to forskolin was seen in control and Aducp2-infected islets (Fig. 2D, P < 0.0001). No differences between control and Aducp2-infected ß-cells were observed at any forskolin concentration. cAMP analogs and insulin secretion
The ability of cell-permeant cAMP analogs 8-Br-cAMP (0.1 mM) and Sp-cAMPs (0.1 mM) to stimulate insulin secretion in ucp2-OE islets was compared with forskolin (1 µM). Both compounds increased insulin secretion in control and ucp2-OE islets (Fig. 2E). To examine PKA-independent effects mediated by epac, 8-pCPT-2-O-Me-cAMP (0.3 mM) was used. Significant effects on control but not ucp2-OE islets were observed (Fig. 2E).
Stimulation of insulin secretion after bypassing KATP channels
The KATP-independent pathway of insulin secretion can be studied by opening KATP channels with diazoxide and depolarizing the ß-cells with KCl. This treatment resulted in the stimulation of insulin secretion in both control and ucp2-OE islets (Fig. 2F). Addition of 1 µM forskolin caused additional stimulation of insulin secretion in both groups (P < 0.01).
KATP channel activity
In the presence of 11 mM glucose, ß-cells from ucp2-OE islets tended to have greater KATP current through KATP channels than control islets (P = 0.15, n = 5–6; Fig. 3A–C). Increased variability in the ucp2-OE group likely reflects different infection efficiencies between preparations. Because ß-cell KATP channels are largely inhibited at 11 mM glucose (Ashcroft & Rorsman 1989, Cook & Ikeuchi 1989) and, thus, the KATP currents are very small, statistical significance was not achieved. Forskolin abrogated this enhancement of KATP current in ucp2-OE islets, diminishing KATP current amplitude to a level similar to that observed in control islets.
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), but had no significant effect in ucp2-OE islets (Fig. 3D). Addition of 1 µM forskolin significantly inhibited 86Rb+ efflux from ucp2-OE islets (Fig. 3D). However, in the presence of the PKA inhibitorH89 (10 µM),the inhibitoryeffects of forskolin on 86Rb+efflux in the ucp2-OE islets were reversed. Calcium flux
Influx of Ca2+ through voltage-dependent Ca2+ channels occurs secondary to the inactivation of KATP channels. Representative traces showing changes in intracellular Ca2+ in ß-TC cells transfected with ucp2 plasmid compared with control cells (Fig. 4A and B) and islet ß-cells (Fig. 4C) are shown. A summary of the results is presented in Table 2. The basal [Ca2+]i was significantly higher in ucp2-OE than control ß-TC cells. Addition of 10 mM glucose invoked an increase in [Ca2+]i that was only 14% of that observed in control cells, consistent with the failure to alter 86Rb+efflux. The increase in [Ca2+]i was identical in ucp2-OE and control ß-TC cells when forskolin was applied (~23%) and the magnitude of the response was similar to that seen when the KATP channels were inactivated with the sulphonylurea tolbutamide. Likewise, exposure of the cells to 50 mM KCl evoked a strong increase in [Ca2+]i of > 250 nM in both control and ucp2-OE conditions. In islet ß-cells, the increase in [Ca2+]i evoked by glucose was reduced by ~50% in ucp2-OE but the response to forskolin was ~75% of control. The difference probably reflects lower transfection efficiency in the primary cells.
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It was previously reported (Lameloise et al. 2001) that culturing clonal ß-cells in the presence of high concentrations of forskolin for ~18 h could inhibit the expression of ucp2, possibly representing an alternative mechanism for its ability to improve GSIS. To determine if effects on gene expression could contribute to improved insulin secretion, in addition to its acute stimulatory effects, rat islets were cultured overnight in the presence of 10 µM forskolin (Fig. 5A). Treatment with forskolin increased ucp2 mRNA expression by ~30% (P < 0.05). Basal insulin secretion was increased ~fivefold in islets cultured in forskolin and 16.5 mM glucose failed to elicit any further augmentation of secretion (Fig. 5B). In contrast, GSIS was threefold basal in the control islets.
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To determine how null expression of ucp2 affects cAMP-potentiated insulin secretion, ucp2 KO mice were utilized. The results of pancreas perfusion experiments are shown in Fig. 6A (WT) and B (ucp2 KO). In the presence of 1.4 mM glucose (1–5 min from Fig. 6A and B), ucp2 KO mice had threefold higher insulin secretion than WT mice. Higher (13.4 mM) glucose evoked a twofold higher response in ucp2 KO than WT mice (Fig. 6C). In WT mice, 1 nM exendin-4 stimulated insulin secretion by fivefold compared with 13.4 mM glucose alone (Fig. 6A and C). Exendin-4 also enhanced insulin secretion from ucp2 KO mouse islets, but by only 1.8-fold (Fig. 6B,C), such that there was no longer any difference in insulin secretion between ucp2 KO and WT mice.
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cAMP, cATP, and cADP contents were measured in freshly isolated ucp2 KO and WT mouse islets. No genotype-dependent difference was observed when cAMP was measured in the presence of glucose alone, 1 nM exendin or 1 µM forskolin (Fig. 6D). However, in the presence of both low and high glucose concentrations, islets from ucp2 KO mice had a higher ATP:ADP ratio than WT mice (Table 3).
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Discussion |
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To study the mechanisms through which cAMP exerts its effects, an abundant source of ß-cells was required. Normal rat islets or ß-TC cells overexpressing UCP2 (Chan et al. 1999, 2001) were utilized. The quantitative PCR results suggest that ucp2 mRNA induction in both models was approximately 20-fold; however, previous work by Joseph et al.(2004) has shown discordance between transcription and translation levels, such that the actual induction of protein is actually two- to fivefold using these transfection or infection methods.
When ß-cell ATP is decreased by ucp2-OE, the ability of glucose to inactivate KATP channels is attenuated (this study and Chan et al. 2001). Similar results were obtained with ucp1-OE in ß-cells (Nakazaki et al. 2002). In contrast, in ucp2 KO mouse islets, glucose-stimulated Ca2+influx is enhanced (Joseph et al. 2005), reflecting increased KATP-dependent depolarization. Therefore, treatments that normalize KATP channel activity and Ca2+ influx should overcome the suppressive effects of UCP2 on GSIS. Here, forskolin reduced KATP currents measured by patch clamping and 86Rb+efflux in ucp2-OE islets and normalized glucose-stimulated Ca2+ influx in response to glucose. The effects of forskolin were largely mediated by PKA because the specific inhibitors H89 and KT5720 (Yaekura et al. 1996) blocked both KATP channel inhibition and insulin secretion, whereas the epac pathway-specific agonist 8-pCPT-2'-O-Me-cAMP (Holz 2004) did not enhance insulin secretion in ucp2-OE islets. Even in control islets, the epac agonist 8-pCPT-2-O-Me-cAMP had only modest effects on insulin secretion compared with forskolin, suggesting that this pathway ‘fine tunes’ insulin secretion through mechanisms not sufficient to over-ride other deficits. cAMPexerts its effects at least partially via KATP channels (Light et al. 2002). Using ß-cell lines, Light et al.(2002) showed that H89 completely blocked the inhibition of KATP currents by GLP-1. The results presented here support the hypothesis that an increase in cAMP can ameliorate insulin secretion despite low cellular ATP via actions on the KATP channel.
These studies also support the potential effects of cAMP on distal events related to exocytosis (Takahashi et al. 1999). Forskolin enhanced insulin secretion by the KATP-independent pathway in both control and ucp2-OE islets. The magnitude of potentiation in depolarized islets was about 30%, whereas total potentiation in non-depolarized islets was 50–100%, suggesting that a significant fraction of cAMP-mediated effectswere exerted on the exocytotic machinery. Exocytosis of insulin can be positively modulated by both PKA and epac (Holz 2004). Since 8-pCPT-2'-O-Me-cAMP was ineffectual in ucp2-OE islets, we speculate that PKA-dependent steps, for example, replenishment of the readily releasable granule pool were contributing to the enhancement of GSIS under these conditions.
An unexpected finding of these studies was the higher basal [Ca2+]i in ucp2-OE ß-cells. The cause of this observation was not investigated but we speculate that lower cellular ATP may lead to sluggish activity of Ca-ATPases that normally sequester Ca2+ in the endoplasmic reticulum or pump it out of the cell. Interestingly, ucp2 KO mice, which have elevated cellular ATP, did not have lower basal [Ca2+]i but after exposure to palmitic acid, which impairs the ability of WT but not ucp2 KO mouse islets to generate ATP, the [Ca2+]i was lower in the ucp2 KO islets (Joseph et al. 2004).
Changes in UCP2 expression did not alter cAMP production in ß-cells. The lack of difference is consistent with kinetic analyses of adenylate cyclase, which showed that the Km for ATP is ~350 µM (Dessauer & Gilman 1997). Resting ATP concentrations in ß-cell cytosolic and plasma membrane domains have been estimated to be ~1000 µM, approximately doubling after high glucose exposure (Kennedy et al. 1999). Thus, even a 50% reduction in ATP should not affect cAMP generation except under exceptional circumstances. Moreover, as the cAMP content increased after forskolin stimulation, the insulin secretion by ucp2-OE islets was normalized. Because PKA activity was similar in control and ucp2-OE islets, it is unlikely that upregulation of this enzyme contributed to the effect. Results from the ob/ob mouse islets showed that in the presence of forskolin a robust insulin response to glucose was generated. Thus, adequate cAMP levels were able to ‘rescue’ energy-deficient islets. Likewise, cAMP is shown to partially relieve the impairment in GSIS observed in the hyperglycemic GK rat (Abdel-Halim et al. 1996). The gene for ucp2 maps within the quantitative trait locus of chromosome 1 for glucose intolerance in the GK rat (Kaisaki et al. 1998), but whether ß-cell ucp2 expression is elevated is unclear. One study showed that the treatment with insulin to normalize glycemia reduced UCP2 protein expression on GK rats fed a high fat diet (Briaud et al. 2002). In neonatal streptozotocin diabetic rats, agents that induce ß-cell cAMP also enhance GSIS, although not to control levels (Dachicourt et al. 1996). Our data, together with other published reports, support the development of new treatment modalities for type-2 diabetes mellitus that target cAMP, such as long-acting stimulants of cAMP production or phosphodiesterase inhibitors (Furman et al. 2004). However, caution against chronic amplification of cAMP-mediated effects is warranted in light of the upregulation of ucp2 mRNA observed in this study and the accompanying exaggerated basal insulin secretion. Agonists that increase cAMP also increased UCP2 expression in muscle cells (Nagase et al. 2001) and activation in dopamine-secreting cells (Yamada et al. 2003), presumably via a cAMP response element in the ucp2 promoter (Yoshitomi et al. 1999). Interestingly, a previous report indicated that 18-h forskolin treatment of rat insulinoma cells (INS-1) reduced ucp2 expression (Lameloise et al. 2001). Differences from our study might be due to the experimental model (transformed cells versus rat islets) and the concentration of forskolin used (fivefold higher than the present study).
Previous studies showed that ucp2 KO mice have an increased insulin-secretory response to both basal and stimulatory glucose concentrations (Zhang et al. 2001, Joseph et al. 2004), a finding confirmed here. When WT mouse pancreases were perfused with stimulatory glucose plus exendin-4, a glucagon-like peptide analog that activates adenylate cyclase to elevate cAMP, insulin secretion was increased by ~fourfold. In comparison, although exendin-4 potentiated GSIS in the ucp2 KO mice, the increment was only ~twofold; thus, the difference in insulin-secreting capacity between the WT and ucp2 KO mice was negated. These data suggest that an abundance of ATP does not lead to any exceptional potentiation of GSIS by cAMP. Rather, the situation appears to resemble that found in the Zucker fatty rat, where a decrease in the Km for glucokinase (Chan 1993, Chan et al. 1995) leads to a left shift in the responsiveness to glucose at both the level of the KATP channel (Chan & MacPhail 1996) and insulin secretion (Chan et al. 1995, 1996). The enhanced inhibition of the KATP channel was presumed due to a greater increment in ATP permitted by the increased glucose flux through glucokinase. Thus, these rats do not display any increased sensitivity to cAMP generating incretins, such as GIP (Chan et al. 1984). Similarly in the diabetic sand rat, any increase in response to incretins or forskolin was attributed to an increase in sensitivity to glucose (Nesher et al. 2001). Of interest, however, was the relatively greater enhancement of the first phase than the second phase of insulin secretion by exendin in ucp2 KO mice. The magnitude of the first phase depends upon the number of granules in the readily releasable pool (Barg et al. 2002) and, in the intact, perfused pancreas, the total ß-cell mass, as well as KATP channel inactivation. KATP channel closure may be enhanced in ucp2 KO mice because of the relatively higher ATP/ADP at low glucose (Joseph et al. 2004). Also, in ucp2 KO mice, ß-cell mass is increased by 50%, but alterations in granule priming and docking in the presence of elevated cAMP cannot be ruled out.
In conclusion, when ß-cell ATP is increased or decreased by manipulating UCP2 expression, different effects on ATP-dependent pathways are observed. Whereas the ability of the KATP channel to close in response to glucose is impaired, cAMP formation is unaltered. This supports the theory that various elements of the secretory pathway have differing energy requirements (Detimary et al. 1994). However, when cAMP concentrations in the islet are elevated, insulin secretion in the ATP-deficient state can be normalized, largely through PKA-dependent mechanisms.
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Acknowledgements |
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Received 4 January 2006
Received in final form 4 May 2006
Accepted 22 May 2006
Made available online as an Accepted Preprint 16 June 2006
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) on glucose (2.8–22.0 mM)-stimulated insulin secretion of islets isolated from (A) lean (n = 14), and (B) ob/ob mice (n = 10). Control islets from each genotype are shown by 
. *P < 0.05, **P < 0.01 and ***P < 0.001 compared with controls.
Significant (P < 0.05) effect of forskolin. (B) Effects of ucp2-OE (solid bars) on forskolin-stimulated cAMP generation in rat islets exposed to 11 mmol/l glucose. Control islets are represented by open bars. n = 5–8. *Significant effect of forskolin (P < 0.05). (C) Effects of specific PKA inhibitors H89 (10 µM) and KT5720 (1 µM) on forskolin (1.0 µM)-stimulated insulin secretion in ucp2-OE rat islets. *P < 0.05 compared with 11 mM glucose (n = at least 9 for all groups). (D) Effects on insulin secretion of cAMP analogs that activate PKA and epac (0.1 mM 8-Br-cAMP, 0.1 mM Sp-cAMPs or 1 µM forskolin) and an epac-specific analog 8-pCPT-2-O-Me-cAMP (0.3 mM). *P < 0.05 compared with 11 mM glucose. n = 6–10. (E) Activity of PKA in islets overexpressing ucp2 (solid bars, n = 5) compared with controls (open bars, n = 6) under basal conditions (0), stimulated with 1 µmol/l forskolin (Forsk) ± H-89 (10 µM). *P < 0.05 compared with basal PKA activity. (F) Insulin secretion via KATP-independent pathway in control and ucp2-OE islets. Islets were held in a depolarized state by addition of 0.1 mM diazoxide and 20 mM KCl in the presence of 11 mM glucose. Forskolin (1 µM) was added to the depolarized islets. *P < 0.05 compared with 2.8 mM glucose, 
