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We investigated the direct effect of a nitric oxide donor (spermine NONOate) on glucose transport in isolated human skeletal muscle and L6 skeletal muscle cells. We hypothesised that pharmacological treatment of human skeletal muscle with N-(2-aminoethyl)-N-(2-hydroxy-2-nitrosohydrazino)-1,2-ethylenediamine (spermine NONOate) would increase intracellular cyclic GMP (cGMP) levels and promote glucose transport.
Skeletal muscle strips were prepared from vastus lateralis muscle biopsies obtained from seven healthy men. Muscle strips were incubated in the absence or presence of 5 mmol/l spermine NONOate or 120 nmol/l insulin. The L6 muscle cells were treated with spermine NONOate (20 µmol/l) and incubated in the absence or presence of insulin (120 nmol/l). The direct effect of spermine NONOate and insulin on glucose transport, cGMP levels and signal transduction was determined.
In human skeletal muscle, spermine NONOate increased glucose transport 2.4-fold (p<0.05), concomitant with increased cGMP levels (80-fold, p<0.001). Phosphorylation of components of the canonical insulin signalling cascade was unaltered by spermine NONOate exposure, implicating an insulin-independent signalling mechanism. Consistent with this, spermine NONOate increased AMP-activated protein kinase (AMPK)-α1-associated activity (1.7-fold, p<0.05). In L6 muscle cells, spermine NONOate increased glucose uptake (p<0.01) and glycogen synthesis (p<0.001), an effect that was in addition to that of insulin. Spermine NONOate also elicited a concomitant increase in AMPK and acetyl-CoA carboxylase phosphorylation. In the presence of the guanylate cyclase inhibitor LY-83583 (10 µmol/l), spermine NONOate had no effect on glycogen synthesis and AMPK-α1 phosphorylation.
Pharmacological treatment of skeletal muscle with spermine NONOate increases glucose transport via insulin-independent signalling pathways involving increased intracellular cGMP levels and AMPK-α1-associated activity.
Nitric oxide is implicated in a wide array of signalling networks . In rodents and humans, exercise increases skeletal muscle nitric oxide production, concomitant with increased glucose uptake [2–4]. Nitric oxide biogenesis is catalysed by different isoforms of nitric oxide synthase (NOS) , of which neuronal-type NOS and endothelial-type NOS isoforms are produced in skeletal muscle . Neuronal-type NOS is produced at higher levels in human skeletal muscle than brain  and therefore is likely to be the major isoform involved in the effect of nitric oxide on glucose metabolism . Acute administration of the NOS inhibitor NG-monomethyl-l-arginine during exercise in humans reduces leg muscle glucose uptake , implicating nitric oxide signalling in the mechanism by which exercise controls glucose homeostasis.
The intracellular mechanism by which nitric oxide increases skeletal muscle glucose uptake in humans is incompletely resolved. Intra-femoral artery infusion of a nitric oxide donor increased glucose uptake in healthy participants , as well as in type 2 diabetic patients . Furthermore, exposure of isolated rat skeletal muscle to the nitric oxide donor sodium nitroprusside increased glucose transport in a dose-dependent manner [9, 10]. Stimulation of glucose transport by nitric oxide involves the activation of a calcium/contraction- and phosphatidylinositol-3-kinase-independent pathway that acutely increases GLUT4 content at the cell surface . Nitric oxide seems to exert its action on muscle glucose transport partly via activation of guanylate cyclase, leading to elevation of cyclic GMP (cGMP) levels [10, 12]. Indeed, the cGMP analogue 8-bromo-cGMP also increases glucose uptake in isolated rat skeletal muscle . Thus, nitric oxide/cGMP signalling may be part of a novel pathway that regulates skeletal muscle glucose uptake.
The effect of exercise on the acute regulation of skeletal muscle glucose transport has been attributed to several signalling nodes including Ca2+-calmodulin-dependent protein kinase (CaMK)II, AMP-activated protein kinase (AMPK) and nitric oxide . In this regard, the interaction between AMPK and nitric oxide signalling pathways is especially intriguing. AMPK is a serine/threonine protein kinase, which acts as a sensor of cellular energy status and regulates a wide variety of gene regulatory and metabolic pathways, including glucose uptake and fatty acid oxidation in skeletal muscle . AMPK subunits (α1, α2, β1, β2, γ1, γ2, γ3) form a heterotrimeric enzyme consisting of α (catalytic), and β and γ (regulatory) isoforms. In rodent skeletal muscle, sodium nitroprusside increases glucose transport, concomitant with α1-associated AMPK activation . Moreover, chronic exposure of L6 muscle cells to sodium nitroprusside increases Glut4 (also known as SLC2A4) mRNA expression by an AMPK-dependent mechanism , positioning AMPK downstream of nitric oxide signalling. AMPK is also considered to be an upstream kinase for NOS, since it phosphorylates and activates endothelial and neuronal NOS [17–19]. Thus, a positive feedback interaction between AMPK and NOS in the control of skeletal muscle metabolism is implicated .
In the present study, we determined the effect of the nitric oxide donor spermine N-(2-aminoethyl)-N-(2-hydroxy-2-nitrosohydrazino)-1,2-ethylenediamine NONOate on glucose transport and intracellular signalling in isolated human skeletal muscle. Using L6 skeletal muscle cells, we also determined whether spermine NONOate and insulin have additive effects on glucose uptake and intracellular signalling. We hypothesised that pharmacological treatment of human skeletal muscle with a compound that increases cGMP levels may promote glucose uptake.
Study participants The study protocol was approved by the regional Ethics Committee at Karolinska Institutet. Informed consent was received from all participants (n=7) before participation. The clinical characteristics of the healthy male volunteers are presented in Table 1. Glucose, insulin and HbA1c values were within the normal range, with no elevation of serum aminotransferase levels. None of the participants used tobacco products or reported taking any medication. The participants were asked to refrain from strenuous exercise for 48 h before the study and to report to the laboratory after an overnight fast.
Muscle biopsy procedure Skeletal muscle (~1 g) was obtained by means of an open biopsy. Biopsies were taken under local anaesthesia (mepivakain chloride 5 mg/ml) from the vastus lateralis portion of the quadriceps femoris muscle . An incision (~4 cm) was made 15 cm above the proximal border of patella and the muscle fascia was exposed. Thereafter, four to five muscle fibre bundles were excised and placed in oxygenated Krebs–Henseleit buffer (KHB), which contained 5 mmol/l glucose, 15 mmol/l mannitol and 0.1% (wt/vol.) BSA (RIA Grade; Sigma, St Louis, MO, USA).
Muscle incubation procedure Smaller skeletal muscle strips were dissected from the biopsy specimen, mounted on Plexiglass clamps (9 mm in width) and incubated in vitro in pregassed (95% O2 and 5% CO2) KHB in a shaking water bath at 35°C for 30 min. The gas phase in the vials was maintained during the incubation procedure. Thereafter, skeletal muscle strips were incubated for 30 min at 35°C in KHB in the absence (basal) or presence of either 5 mmol/l spermine NONOate (Calbiochem, San Diego, CA, USA) or 120 nmol/l insulin (Insulin Actrapid; Novo Nordisk, Bagsværd, Denmark). The concentrations of spermine NONOate and insulin were maintained throughout all remaining incubation procedures.
Glucose transport Skeletal muscle strips were transferred to fresh KHB containing 20 mmol/l mannitol and incubated at 35°C for 10 min. Thereafter, muscles were incubated for 20 min in KHB containing 5 mmol/l 3-O-methyl [3H]glucose (29.6 MBq/mmol) and 15 mmol/l [14C]mannitol (2.0 MBq/mmol). Thus, muscle strips were exposed to either spermine NONOate or insulin for a total of 60 min. At the end of the incubation protocol, skeletal muscle specimens were blotted of excess fluid, snap-frozen in liquid nitrogen and stored at −80°C until further analysis. Glucose transport was determined by the accumulation of intracellular 3-O-methyl-[3H]glucose as previously described .
Cyclic guanosine monophosphate measurement Skeletal muscle strips were incubated in the absence or presence of spermine NONOate as described above for 60 min and then rapidly clamp frozen in liquid N2 cooled tongs. Frozen muscles were homogenised on ice in 1 ml 10% (vol./vol.) trichloroacetic acid using a polytron. Homogenates were subjected to centrifugation for 10 min at 14,000 g. Thereafter, the trichloroacetic acid was extracted from the supernatant fraction with 2H2O-saturated diethyl ether. Samples were then immediately frozen in liquid N2 and concentrated in a speed vacuum. The concentrated samples were resuspended in assay buffer and acetylated, after which cGMP levels were measured by immunoassay according to manufacturer’s instructions (cGMP BioTRAK, RPN 226; Amersham, Pittsburgh, PA, USA). cGMP is expressed as pmol/g wet weight.
AMP kinase activity Muscles were homogenised in ice-cold lysis buffer containing 50 mmol/l Tris–HCl (pH 7.5), 1 mmol/l EDTA, 1 mmol/l dithiothreitol, 10% (vol./vol.) glycerol, 50 mmol/l NaF, 5 mmol/l Na pyrophosphate, 1 mmol/l benzamidine, 0.1 mmol/l phenylmethyl sulfonyl fluoride and 1% (vol./vol.) Triton X-100. Muscle homogenates were subjected to centrifugation for 10 min at 14,000 g and 4°C. Supernatant fractions were removed and used to determine protein content using a commercially available kit based on the Bradford method (Bio-Rad, Hercules, CA, USA). Aliquots (200 μg protein) were incubated overnight at 4°C with antibodies against α1- and α2-AMPK subunits (provided by D. G. Hardie, Division of Molecular Physiology, College of Life Sciences, University of Dundee, Dundee, UK). Human muscle lysates from rested and exercised conditions were also incubated overnight at 4°C with antibodies against the AMPK-α1- and α2-subunits, and were used as positive control for the assay. The immunoprecipitates were washed once in lysis buffer, once in 480 mmol/l HEPES (pH 7.0) and 240 mmol/l NaCl, and twice in 240 mmol/l HEPES (pH 7.0) and 120 mmol/l NaCl, leaving 10 µl of buffer with the Sepharose after the last wash. To determine isoform-specific AMPK activity, the immunoprecipitates were incubated for 30 min at 30°C in a total volume of 30 µl containing 833 µmol/l diothiothreitol, 200 µmol/l AMP, 100 µmol/l AMARA-peptide (Upstate Millipore, Billerica, MA, USA), 5 mmol/l MgCl2, 200 µmol/l ATP and 74 kBq of [γ-32P]ATP. The reaction was stopped by spotting 25 µl on to a piece of P81 filter paper, which was then washed four times at 15 min per time in 1% (vol./vol.) phosphoric acid. The dried filter paper was analysed for activity using liquid scintillation counting.
Cell culture L6 muscle cells (provided by A. Klip, The Hospital for Sick Children, Toronto, ON, Canada) were grown in αMEM supplemented with 10% (vol./vol.) FBS, 1% (vol./vol.) penicillin and streptomycin (100 U/ml penicillin, 100 µg/ml streptomycin), and 1% (vol./vol.) fungizone in 5% CO2 95% O2 humidified air at 37°C. The L6 cells were differentiated into myotubes for 6 days in αMEM supplemented with 2% (vol./vol.) FBS. Myotubes were then serum-starved for 3 h before the start of the experiment. Myotubes were incubated under basal conditions or in the presence or absence of spermine NONOate (20 µmol/l) or a guanylate cyclase inhibitor (10 µmol/l LY-83583) and glucose incorporation into glycogen (glycogen synthesis), glucose uptake and protein signalling were determined. To establish insulin-stimulated conditions, insulin (120 nmol/l) was added during the last 20 min for protein phosphorylation and glucose uptake analysis or during the last 120 min for glycogen synthesis analysis.
Glucose incorporation to glycogen (glycogen synthesis) Glycogen synthesis was assessed in L6 cells by measuring the incorporation of d-[U-14C]glucose into glycogen as described . Overnight serum-starved myotubes were incubated in 6 well plates and treated for 1 h with spermine NONOate (20 µmol/l) and LY-83583 (10 µmol/l), in the absence or presence of insulin (120 nmol/l). During the last 90 min, the cells were incubated with medium supplemented with glucose (5 mmol/l) and d-[U-14C]glucose (final specific activity, 37 kBq/ml). Each experiment was performed on duplicate wells. Glucose uptake and incorporation to glycogen was determined as mmol glucose per mg protein per h.
Glucose uptake Myotubes were serum-starved for 3 to 5 h and incubated with or without spermine NONOate (20 µmol/l) in the absence or presence of insulin (120 nmol/l). 2-Deoxyglucose uptake was determined as described . Each experiment was performed on duplicate wells.
Western blot analysis A portion of the muscle specimen incubated for the glucose transport assay was homogenised in 0.3 ml ice-cold lysis buffer using a glass-on-glass system with a motor pestle. The buffer contained 20 mmol/l Tris (pH 8.0), 137 mmol/l NaCl, 2.7 mmol/l KCl, 10 mmol/l NaF, 1 mmol/l MgCl2, 1 mmol/l Na3VO4, 0.2 mmol/l phenylmethylsulfonyl fluoride, 10% (wt/vol.) glycerol, 1% (wt/vol.) Triton X-100, 1 µg/ml aprotinin, 1 µg/ml leupeptin and 1 μmol/l microcystin. L6 myotubes were collected into similar ice-cold lysis buffer. Homogenates were solubilised by end-over-end mixing for 60 min at 4°C and subjected to centrifugation (for 10 min at 4°C and 12,000 g). The supernatant fraction was stored at −80°C until use. Total protein was determined using a commercially available kit (Pierce, Rockford, IL, USA). Equal amounts of protein (40 µg) were diluted in Laemmli sample buffer. Proteins were separated by SDS–PAGE and transferred to membranes (Immobilon-P; Millipore). Phosphorylation and levels of several proteins were determined using the following antibodies: phospho-AMPK Thr172, phospho-Akt Ser473, phospho-Akt-substrate (PAS), phospho-glycogen synthase kinase (GSK)-α/β (Ser21/9) and phospho-CaMKII Thr286 (all from Cell Signaling Technology, MA, USA), phospho-ACCβ Ser227 and ACC (Upstate Biotechnologies, MA, USA) and GLUT4 (Chemicon, CA, USA). Anti-α1-AMPK and anti α2-AMPK antibodies used for the immunoblot analysis were kindly provided by D. G. Hardie (Division of Molecular Physiology, College of Life Sciences, University of Dundee, UK). All membranes were normalised for loading with glyceraldehyde-3-phosphate dehydrogenase (Santa Cruz Biotechnology, Santa Cruz, CA, USA) or respective total protein content. Proteins were visualised by chemiluminescence and quantified by densitometry.
Statistics Data are reported as mean ± SE. Differences were determined using a paired t test or ANOVA as appropriate. Bonferroni test was used for post hoc analysis. Significance was established at p<0.05.
Effects of spermine NONOate on glucose transport and AMP kinase activity We determined the effects of spermine NONOate and insulin on glucose transport in intact human skeletal muscle (Fig. 1a). Muscle strips were incubated in the absence or presence of either 5 mmol/l spermine NONOate or 120 nmol/l insulin and 3-O-methyl-glucose transport was assessed. Insulin increased glucose transport fivefold (p<0.05) in isolated skeletal muscle strips, consistent with our earlier studies . Spermine NONOate increased skeletal muscle glucose transport 2.4-fold (p<0.05), concomitant with increased cGMP levels (p<0.001) (Fig. 1b). AMPK activation has been implicated in the mechanism by which nitric oxide enhances glucose uptake in skeletal muscle . Thus, we determined the effects of spermine NONOate exposure on α-isoform-specific AMPK signalling (Fig. 1c, d). For perspective, acute exercise increased AMPK-α1- and AMPK-α2-associated activity in skeletal muscle from healthy men by two- and 6.2-fold, respectively vs rested conditions (Fig. 1e, f). Spermine NONOate increased AMPK-α1-associated activity 1.7-fold (p<0.05), while AMPK-α2-associated activity was unchanged in isolated skeletal muscle. Previous studies from our laboratory provide evidence that insulin does not alter AMPK-α1- or AMPK-α2-associated activity in isolated human skeletal muscle .
Effects of spermine NONOate on protein content and signal transduction The effects of insulin or spermine NONOate on canonical insulin signalling were determined in isolated skeletal muscle using phospho-specific antibodies (Fig. 2a). Exposure of human skeletal muscle to insulin increased the phosphorylation of Akt (Ser473), Tre-2/BUB2/CDC16 domain-containing protein family, member 1, domain family 1/domain family 4 (pTBC1D1/D4) (detected using a PAS antibody) and GSK3α/β (Ser21/9), while spermine NONOate had no effect (Fig. 2a–d). Neither insulin nor spermine NONOate treatment altered CaMK signalling, since phosphorylation of CaMKII (Thr286) was unaltered compared with non-stimulated (basal) muscle (Fig. 2e). Abundance of the AMPK-α1 and AMPK-α2 subunits in isolated skeletal muscle was unaltered after 1 h exposure of isolated skeletal muscle to spermine NONOate or insulin (Fig. 2a). In L6 cells, nitric oxide is known to increase GLUT4 levels via an AMPK-dependent mechanism . GLUT4 content was unaltered after 1 h exposure of isolated skeletal muscle to spermine NONOate or insulin (data not shown), suggesting spermine NONOate acutely increases glucose transport in muscle by recruiting existing glucose transporters to the cell surface, rather than through GLUT4 biogenesis.
Effect of spermine NONOate and insulin on glycogen synthesis and glucose uptake To determine whether spermine NONOate and insulin have an additive effect on glucose metabolism, we measured glucose incorporation into glycogen (glycogen synthesis) (Fig. 3a) and glucose uptake (Fig. 3b) in L6 myotubes. Spermine NONOate and insulin increased glycogen synthesis 1.2- (p<0.001) and 2.2-fold (p<0.0001), respectively (Fig. 3a). Combined exposure to spermine NONOate and insulin had an additive effect on glycogen synthesis. Similarly, spermine NONOate and insulin independently increased glucose uptake 1.2- (p<0.01) and 1.2-fold (p<0.001) (Fig. 3b). Combined exposure to spermine NONOate and insulin also had an additive effect on glucose uptake. To delineate underlying mechanism for the additive effect on glucose uptake and metabolism, phosphorylation of AMPK, ACC, Akt and TBC1D1/D4 was measured (Fig. 3c–f). Spermine NONOate alone increased phosphorylation of AMPK Thr172 6.3-fold (p<0.05) and pACC Ser227 1.7-fold (p<0.05), while insulin alone had no effect. Interestingly, phosphorylation of AMPK Thr172 and pACC Ser227 was unaltered in the presence of spermine NONOate and insulin. Nevertheless, insulin led to a 6.5-fold increase in Akt Ser473 phosphorylation (p<0.05) and a 3.5-fold increase in TBC1D1/D4 phosphorylation (p<0.05), these responses being unaltered in presence of spermine NONOate. Finally, phosphorylation of Akt Ser473 and TBC1D1/D4 was unaltered in the presence of spermine NONOate.
Effect of the guanylate cyclase inhibitor LY-83583 on spermine NONOate-induced glycogen synthesis and AMPK phosphorylation An earlier report provides evidence that LY-83583 inhibits guanylate cyclase activity . Since spermine NONOate exposure increased AMPK-α1-associated activity in human skeletal muscle (Fig. 1c), as well as phosphorylation of AMPK and ACC in L6 myotubes (Fig. 3c, e), we determined whether AMPK activation lies downstream of cGMP. Treatment of L6 myotubes with spermine NONOate increased glycogen synthesis and AMPK Thr172phosphorylation, but these responses were abolished in the presence of LY-83583 (10 µmol/l) (Fig. 4a, b). However, LY-83583 (10 µmol/l) increased glycogen synthesis in L6 myotubes (p<0.001). This dose was selected for our in vitro studies on the basis of a previous report . Treatment of L6 myotubes with a lower concentration of LY-83583 (100 nmol/l) also increased glycogen synthesis (data not shown). Importantly, we provide evidence that only the α1 subunit of AMPK is present in L6 myotubes, since immunoblot analysis failed to detect the α2 subunit of AMPK (Fig. 4c).
Regular exercise training improves glucose tolerance  and skeletal muscle insulin sensitivity  in type 2 diabetic patients, but the molecular mechanisms are incompletely resolved. Although several strategies designed to enhance compliance with physical activity regimens in patients with insulin resistance have been proposed , many type 2 diabetic patients rely on pharmacological treatments to improve glucose homeostasis. Yet, these current pharmacological treatments to enhance peripheral insulin sensitivity have limited efficacy . Therefore, insight into novel mechanisms capable of enhancing skeletal muscle glucose uptake could lead to new pharmaceutical strategies to improve treatment and possibly prevent peripheral insulin resistance in patients with type 2 diabetes.
Nitric oxide signalling plays a key role in exercise/contraction-induced metabolic responses in skeletal muscle , partly via an AMPK-dependent mechanism . During exercise/contraction, increased nitric oxide levels are associated with induction of glucose uptake in skeletal muscle [2–4]. Conversely, NOS inhibition reduces glucose uptake during exercise in type 2 diabetic patients more than in control participants . Previous reports characterising the direct effects of nitric oxide on glucose uptake are limited to in vitro studies of isolated rodent skeletal muscle [9–11]. Here we provide evidence that pharmacological treatment of human skeletal muscle with the nitric oxide donor spermine NONOate increases glucose transport, concomitant with increased cGMP levels and AMPK-α1-associated activity. Using L6 myotubes (producing only the α1-subunit of AMPK), we provide evidence that spermine NONOate increases phosphorylation of AMPK and ACC, with a concomitant increase in glucose transport and glycogen synthesis. Our findings in human skeletal muscle are compatible with earlier studies in rodent muscle indicating that nitric oxide donors increase cGMP levels and glucose transport . Similar effects on glucose transport stimulation were also observed in isolated rat skeletal muscle exposed to the cGMP analogues 8-bromo-cGMP  and dibutyryl cGMP . The mechanism by which cGMP regulates glucose uptake may involve two enzymes, namely guanylate cyclase and phosphodiesterase, but other mechanisms are also likely to be involved. Inhibition of guanylate cyclase prevents the sodium nitroprusside-induced increase in cGMP levels and glucose transport . Conversely, treatment of isolated skeletal muscle with a phosphodiesterase inhibitor (Zaprinast) increases cGMP levels, with a concomitant increase in glucose uptake . Collectively, these studies provide evidence that the nitric oxide/cGMP pathway is likely to be important in the regulation of glucose transport.
Nitric oxide signalling has been linked to AMPK activation and glucose uptake [15, 16]. Here, we provide evidence that in vitro exposure to a nitric oxide donor increases glucose transport, with concomitant increase in AMPK-α1-specific activity and AMPK-α1 phosphorylation in isolated human skeletal muscle and L6 myotubes. Among the 12 possible AMPK heterotrimers, only three (α1β2γ1, α2β2γ1, α2β2γ3) have been identified in human skeletal muscle . Each individual heterotrimer is activated in a manner dependent on time and intensity [34, 35], which may elicit signalling specificity in response to a distinct set of stimuli. Our results in human skeletal muscle and L6 myotubes provide evidence that nitric oxide specifically increases AMPK-α1-associated activity and AMPK-α1 phosphorylation respectively. Moreover in L6 myotubes, the guanylate cyclase enzyme inhibitor LY-83583 prevents the nitric oxide donor-induced increase in glycogen synthesis and α1-AMPK phosphorylation, providing evidence for a potential role of the AMPK-α1 subunit in the mechanism by which nitric oxide donors increase glucose transport. These observations are consistent with a previous study in rodent skeletal muscle , which provided evidence that sodium nitroprusside increases AMPK-α1-, but not AMPK-α2-associated activity. Furthermore, in rodent skeletal muscle, sodium nitroprusside-induced increases in AMPK-isoform-specific activity occurred independently of changes in ATP, creatinine phosphate or glycogen levels . Thus, the nitric oxide–cGMP pathway may be involved in the regulation of AMPK-α1 activity and/or inhibition of the protein phosphatase responsible for AMPK regulation.
Although most Ampk (also known as Prkaa2) knockout models provide evidence against a critical role for the AMPK-α1 subunit in the regulation of skeletal muscle glucose uptake , AMPK-α1 activation is required for stimulation of glucose uptake in response to twitch contraction . Based on our results, the promotion of glucose uptake effected by the nitric oxide donor appears to be at least partly mediated via AMPK complexes containing the α1 subunit. However, the role of AMPK in nitric oxide signalling is complex, since AMPK has also been suggested to be an upstream kinase for NOS [17–19, 37]. Direct activation of AMPK, using 5′-aminoimidazole-4-carboxamide ribonucleoside (AICAR), stimulates nitric oxide production in human aortic endothelial cells  and increases NOS activity in H-2Kb cells , implicating a feedback loop between AMPK and NOS . The question of whether nitric oxide pathways lie upstream or downstream of AMPK remains unresolved. For example, AICAR-induced AMPK-activated glucose transport is unaltered by NOS inhibition in isolated rat skeletal muscle . The direct interaction between the nitric oxide/cGMP pathway and AMPK warrant further investigation.
To determine the intracellular mechanism by which the nitric oxide donor spermine NONOate increases glucose transport, components of the canonical insulin signalling cascade were assessed. The Akt- and Rev/Rex activation domain-binding protein (Rab) GTPase-activating proteins, TBC1D1 and TBC1D4, are the most distal signalling proteins implicated in GLUT4 translocation [39, 40]. In human skeletal muscle, insulin exposure led to an expected increase in phosphorylation of Akt, TBC1D1/D4 (detected using a PAS antibody) and GSK3, while exposure to the nitric oxide donor had no effect. These data indicate that nitric oxide-stimulated glucose transport is mediated via an insulin-independent pathway. Nitric oxide has also been linked as a positive  modulator of GLUT4 production. However, GLUT4 protein content was unaltered in response to spermine NONOate (data not shown), presumably because of the shorter incubation time and low concentration of the nitric oxide donor used in this study. CaMKII signalling has been implicated in the mechanism by which muscle contraction increases glucose uptake . Nevertheless, CaMKII phosphorylation was unaltered in response to insulin or spermine NONOate. In contrast to our results for AMPK signalling, insulin and CaMKII signalling do not appear to play a role in nitric oxide action on skeletal muscle glucose transport. In L6 myotubes, the nitric oxide donor and insulin had an additive effect on glycogen synthesis and glucose uptake without further increase in insulin-induced Akt and TBC1D1/D4 phosphorylation. These results suggest that nitric oxide promotes glucose uptake by an insulin-independent mechanism. Furthermore, the stimulatory effect of the nitric oxide donor on AMPK and ACC phosphorylation under insulin-stimulated conditions was prevented, excluding a role for AMPK signalling in the additive effect on glycogen synthesis and glucose uptake.
In summary, the nitric oxide donor spermine NONOate increases cGMP levels and promotes glucose transport, concomitantly with AMPK-α1-isoform-specific activation in human skeletal muscle. Further study to delineate mechanisms and the therapeutic window is warranted. Spermine NONOate also increased glucose transport in L6 myotubes, concomitantly with an increase in AMPK-α1-isoform-specific phosphorylation. Moreover, these effects were prevented in presence of a guanylate cyclase inhibitor. Further studies on the mechanisms by which AMPK-α1-isoform-specific signalling is directly linked to nitric oxide action are warranted. Taken together with recent evidence showing that sodium nitroprusside increased glucose uptake in human primary myotubes derived from healthy volunteers and patients with type 2 diabetes , our findings have clear clinical implications, since manipulation of the nitric oxide/cGMP signalling cascade could enhance glucose uptake by an insulin-independent mechanism to potentially improve whole-body glucose homeostasis in type 2 diabetic patients.
This work was supported by grants from the European Research Council, the Swedish Research Council, the Swedish Diabetes Association, Novo Nordisk Foundation, the Foundation for Scientific Studies of Diabetology, the Swedish Centre for Sports Research, the Strategic Research Foundation, the Commission of the European Communities (Contract numbers LSHM-CT-2004-005272 EXGENESIS and LSHM-CT-2004-512013 EUGENE2). Additional support to H. A. Koistinen was provided by grants from Finnish Academy of Science and Sigrid Juselius Foundation.
Duality of interest The authors declare that there is no duality of interest associated with this manuscript.
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