Clenbuterol exerts antidiabetic activity through metabolic reprogramming of skeletal muscle cells

Meister, Jaroslawna; Bone, Derek B. J.; Knudsen, Jonas R.; Barella, Luiz F.; Velenosi, Thomas J.; Akhmedov, Dmitry; Lee, Regina J.; Cohen, Amanda H.; Gavrilova, Oksana; Cui, Yinghong; Karsenty, Gerard; Chen, Min; Weinstein, Lee S.; Kleinert, Maximilian; Berdeaux, Rebecca; Jensen, Thomas E.; Richter, Erik A.; Wess, Jürgen

doi:10.1038/s41467-021-27540-w

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Published: 10 January 2022

Clenbuterol exerts antidiabetic activity through metabolic reprogramming of skeletal muscle cells

Nature Communications volume 13, Article number: 22 (2022) Cite this article

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Abstract

Activation of the sympathetic nervous system causes pronounced metabolic changes that are mediated by multiple adrenergic receptor subtypes. Systemic treatment with β_2-adrenergic receptor agonists results in multiple beneficial metabolic effects, including improved glucose homeostasis. To elucidate the underlying cellular and molecular mechanisms, we chronically treated wild-type mice and several newly developed mutant mouse strains with clenbuterol, a selective β₂-adrenergic receptor agonist. Clenbuterol administration caused pronounced improvements in glucose homeostasis and prevented the metabolic deficits in mouse models of β-cell dysfunction and insulin resistance. Studies with skeletal muscle-specific mutant mice demonstrated that these metabolic improvements required activation of skeletal muscle β₂-adrenergic receptors and the stimulatory G protein, G_s. Unbiased transcriptomic and metabolomic analyses showed that chronic β₂-adrenergic receptor stimulation caused metabolic reprogramming of skeletal muscle characterized by enhanced glucose utilization. These findings strongly suggest that agents targeting skeletal muscle metabolism by modulating β₂-adrenergic receptor-dependent signaling pathways may prove beneficial as antidiabetic drugs.

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Introduction

The number of people suffering from type 2 diabetes (T2D) and impaired glucose tolerance, a major risk factor for the development of T2D, continues to rise in an alarming manner worldwide (IDF Diabetes Atlas, 9th edn. Brussels, Belgium: 2019). Current non-insulin therapies of T2D focus mostly on targeting β-cell dysfunction (GLP-1 mimetics, DPP-4 inhibitors, sulfonylureas, and meglitinides), hepatic and adipose tissue insulin resistance (metformin and thiazolidinediones, respectively), and elimination of excess glucose through the kidneys or gut (SGLT2 and α-glucosidase inhibitors, respectively)¹.

At present, antidiabetic drugs that directly target skeletal muscle (SKM) are not available, even though SKM is responsible for 80–90% of glucose disposal during a euglycemic-hyperinsulinemic clamp in healthy individuals². Moreover, SKM insulin resistance is a key metabolic defect in the pathogenesis of T2D². For these reasons, SKM is a very attractive target for the development of novel classes of antidiabetic drugs. G protein-coupled receptors (GPCRs) represent a highly druggable class of cell surface proteins. In fact, ~35% of all approved pharmaceuticals target specific GPCRs³. SKM expresses dozens of different GPCRs endowed with distinct G protein-coupling properties⁴. In vitro studies have shown that activation of G_q-coupled GPCRs can regulate glucose uptake into SKM cells^5,6,7. By using DREADD (Designer Receptor Exclusively Activated by a Designer Drug) technology, we recently demonstrated that receptor-mediated activation of G_q signaling in SKM tissue in vivo leads to greatly improved glucose tolerance⁸.

Clenbuterol is a synthetic, highly selective β₂-adrenergic receptor (β₂-AR) agonist that is approved for the treatment of asthma and chronic obstructive pulmonary disease in several European and Asian countries (http://drugapprovalsint.com/clenbuterol/). Similar to the β₁- and β₃-AR subtypes, the β₂-AR primarily activates the stimulatory G protein G_s, leading to increased intracellular cAMP levels and the activation of protein kinase A(PKA) and other cAMP-dependent effector proteins⁹. However, several studies have shown that β₂-AR can also modulate cellular signaling via stimulation of cAMP inhibitory G_i-type G proteins^10,11,12. Moreover, activated β₂-ARs, such as other GPCRs, can recruit β-arrestins (β-arrestin-1 and -2), which can also act as signaling proteins^13,14,15.

β₂-ARs are expressed at high levels in SKM, and clenbuterol and other β₂-AR agonists have been reported to prevent or reverse muscle wasting or weakness by promoting SKM growth^16,17. Interestingly, treatment of rodents with clenbuterol has been shown to improve glucose homeostasis^18,19,20. However, the β₂-AR is not only expressed in SKM, but also in many metabolically important tissues, including pancreatic islets and adipose tissues^21,22. For these reasons, it remains unclear which tissues or cell types, and which cellular signaling pathways are involved in mediating the metabolically beneficial actions of clenbuterol in vivo. Specifically, the role of β₂-ARs in regulating SKM glucose fluxes remains controversial. Although some studies reported β₂-AR-mediated inhibition of glucose uptake into SKM^23,24,25,26, other studies reported the opposite effect (stimulation of glucose uptake)^18,20,24,27.

In this study, by analyzing several newly developed mouse models, we demonstrate that the beneficial metabolic effects of chronic clenbuterol are mediated by activation of SKM β₂-ARs, and that the coupling of these receptors to SKM G_s is essential for the manifestation of these clenbuterol effects. In agreement with these findings, selective activation of SKM G_s signaling by a G_s-coupled designer GPCR caused similar improvements in glucose homeostasis. Moreover, unbiased metabolomic and RNA-sequencing (RNA-Seq) studies shed light on the molecular mechanisms underlying the clenbuterol-induced improvements in SKM glucose homeostasis following β₂-AR stimulation. These findings are of considerable relevance for the development of novel antidiabetic drugs targeting SKM glucose metabolism.

Results

Clenbuterol treatment improves whole-body glucose homeostasis in healthy lean mice and mouse models of β-cell dysfunction and insulin resistance

To study the metabolic consequences of chronic stimulation of β₂-ARs in vivo, we administered clenbuterol in drinking water (30 mg/l) to wild-type (WT) mice for 5 days, followed by a series of metabolic tests. Clenbuterol treatment of lean male and female WT mice led to improved glucose tolerance (Fig. 1a and Supplementary Fig. 1a). During an insulin tolerance test (ITT), lean WT mice treated with clenbuterol showed lower blood glucose levels (Fig. 1b). However, when taking into account the significantly lower basal blood glucose levels in the clenbuterol-treated mice, the insulin-mediated decrease in blood glucose levels was similar to that in the control group (Fig. 1b and Supplementary Fig. 1b). Fasting insulin levels were significantly lower following clenbuterol administration, whereas glucose-stimulated insulin secretion (GSIS) remained essentially unchanged (Fig. 1c). Importantly, clenbuterol treatment lowered blood glucose levels and improved glucose tolerance in high-fat diet (HFD)-induced obese mice (Fig. 1d, e) without improving insulin sensitivity (Fig. 1e and Supplementary Fig. 1c).

**Fig. 1: Chronic clenbuterol administration improves glucose tolerance in mice in a SKM-β₂-AR-dependent manner.**

To mimic the loss of β-cell mass characteristic for advanced β-cell dysfunction, we used a streptozotocin (STZ) treatment protocol known to destroy about 70–80% of mouse β-cells²⁸. Specifically, lean WT mice were injected with STZ (50 mg/kg intraperitoneally (i.p.)) for 5 consecutive days. Seven days after the last STZ injection, the mice developed characteristic signs of β-cell dysfunction including elevated fasting and fed blood glucose levels (Supplementary Fig. 1d), decreased plasma insulin concentrations (Supplementary Fig. 1e), reduced body weight (Supplementary Fig. 1f), and impaired glucose tolerance (Supplementary Fig. 1g).

Following 5-day clenbuterol administration, STZ-treated mice showed similar metabolic improvements (Fig. 1f and Supplementary Fig. 1h–j) as seen with lean and obese WT mice (Fig. 1a–e). As our data suggested that altered release of insulin does not contribute to the beneficial metabolic effects of clenbuterol treatment (Fig. 1c and Supplementary Fig. 1j) and β₂-ARs are not expressed in adult mouse hepatocytes²⁹, we speculated that the beneficial effects of clenbuterol on glucose homeostasis (Fig. 1a, d, f) were caused by activation of SKM G_s signaling through SKM β₂-ARs. To test this hypothesis, we generated mice that lacked β₂-ARs or Gα_s selectively in SKM (SKM-β₂-AR-KO and SKM-Gs-KO mice, respectively). The SKM-selective deletion of the β₂-AR and Gα_s was induced in adult mice via tamoxifen-dependent activation of Cre recombinase in SKM only. Efficient deletion of β₂-AR and Gα_s in SKM was confirmed via quantitative real-time PCR (qRT-PCR) or western blotting, respectively (Supplementary Fig. 1k, p). The remaining SKM expression of β₂-ARs and Gα_s displayed by the knockout (KO) mice may be due to the fact that SKM tissue does not only consist of myocytes but also harbors several other cell types³⁰. The lack of SKM β₂-ARs in lean mice did not lead to any obvious metabolic phenotypes (Supplementary Fig. 1l–o). In contrast, lean SKM-Gs-KO showed a significant impairment in glucose tolerance (but normal insulin sensitivity), as compared to their control littermates (Supplementary Fig. 1q–t).

Next, we treated SKM-β₂-AR-KO and SKM-Gs-KO mice for 5 days with clenbuterol (via the drinking water). Remarkably, in the absence of SKM β₂-ARs or SKM Gα_s, the ability of clenbuterol treatment to improve glucose tolerance was abolished (Fig. 1g, h). These data clearly indicate that clenbuterol administration improves whole-body glucose homeostasis by stimulation of SKM β₂-ARs and subsequent activation of SKM G_s.

Multiple studies have shown that chronic administration of clenbuterol over a period of weeks increases SKM mass in various species¹⁶, raising the possibility that changes in SKM growth or mass may contribute to the beneficial metabolic effects of clenbuterol. To examine whether our 5-day clenbuterol treatment protocol resulted in an increased SKM mass, we studied mouse body composition using EchoMRI. We found that body weight (Supplementary Fig. 2a), lean mass (Supplementary Fig. 2b), and fat mass (Supplementary Fig. 2c) were not significantly affected by our clenbuterol treatment protocol. Moreover, the clenbuterol-induced improvement in glucose tolerance could already be observed as early as 36 h after initiation of clenbuterol administration (Supplementary Fig. 2d), whereas insulin secretion was unaltered (Supplementary Fig. 2e). These results suggest that the metabolic improvements of whole-body glucose homeostasis observed after several days of clenbuterol treatment are independent of changes in SKM mass.

Chronic CNO stimulation of SKM G_s DREADD mice (GsD mice) mimics the metabolic improvements seen with clenbuterol-treated WT mice

As β₂-ARs are widely expressed, we took advantage of DREADD technology to clearly define the role of chronic SKM G_s stimulation in regulating glucose homeostasis. DREADDs are mutant GPCRs that are insensitive to any endogenous ligands, but are selectively activated by otherwise pharmacologically inert synthetic agents, such as clozapine-N-oxide (CNO). During the past decade, DREADDs have been successfully used to study cell type-specific metabolic consequences of activating different functional classes of G proteins³¹.

To explore the in vivo metabolic effects caused by chronic stimulation of a G_s-linked GPCR in SKM, we generated mice that expressed a G_s-coupled DREADD (GsD)^{32,33,34,35,36} under the transcriptional control of the SKM-specific human α-skeletal actin (HSA) promoter. We refer to these mice from hereon simply as SKM-GsD mice. In the absence of CNO, male and female SKM-GsD mice did not show any significant changes in glucose homeostasis, as compared to their control littermates (Supplementary Fig. 3a–f).

To further support the concept that activation of receptor-mediated G_s signaling in SKM causes pronounced metabolic improvements, control and SKM-GsD mice maintained on regular chow were treated with CNO (250 mg/l) via the drinking water for 1 week and then subjected to a series of metabolic tests. At the end of the CNO treatment period, male (Fig. 2a) and female (Supplementary Fig. 3g) SKM-GsD mice showed improved glucose tolerance and reduced fasting blood glucose levels (Supplementary Fig. 3h) without changes in body weight (Supplementary Fig. 3i), insulin tolerance (Fig. 2b), GSIS, and plasma insulin levels (Fig. 2c and Supplementary Fig. 3j). Importantly, CNO treatment also improved glucose homeostasis in HFD-induced obese mice (Fig. 2d and Supplementary Fig. 3l). As observed with lean SKM-GsD mice, CNO treatment of obese SKM-GsD mice had no significant effect on body weight (Supplementary Fig. 3k), insulin tolerance and GSIS (Fig. 2e, f, respectively). Thus, the metabolic phenotype observed with SKM-GsD mice treated with CNO closely mimicked the metabolic changes displayed by WT mice after clenbuterol treatment. Taken together, these findings strongly indicate that the metabolic improvements caused by clenbuterol treatment (Fig. 1) depend on the activation of G_s signaling in SKM (Fig. 2).

**Fig. 2: Chronic CNO treatment of SKM-Gs-DREADD mice improves glucose tolerance by enhancing glucose uptake into SKM.**

To investigate whether CNO treatment of SKM-GsD mice led to improved glucose uptake into SKM, we performed in vivo glucose uptake studies using [¹⁴C]-2-deoxyglucose (DG) as a tracer. We found that CNO-treated SKM-GsD mice showed a significant increase of glucose uptake into multiple SKM tissues (quadriceps and gastrocnemius muscles) (Fig. 2g). No changes in glucose uptake were observed in adipose tissues or the brain (Fig. 2g).

Clenbuterol treatment increases glucose utilization in SKM

To explore the changes in SKM cell metabolism following long-term clenbuterol treatment, we used unbiased high-throughput metabolomics and transcriptomics approaches. Metabolomic analysis of SKM (quadriceps muscle) from lean WT mice treated with clenbuterol or regular water identified a total of 648 metabolites. Principal component analysis showed a clear separation of the two experimental groups based on their biochemical profile (Supplementary Fig. 4a). Clenbuterol treatment affected the SKM metabolites of all macronutrient classes (Supplementary Fig. 4b and Supplementary Data 1), leading to changes in the levels of glucose metabolites (Fig. 3a–d, i), lipids (Fig. 4f and Supplementary Fig. 5g), ketone bodies (Supplementary Fig. 5c), and amino acids (Supplementary Fig. 6a, b). In agreement with these extensive changes in metabolite levels, transcriptome analysis identified >4000 differentially expressed genes that are involved in multiple metabolically relevant pathways (Supplementary Fig. 4c).

**Fig. 3: Chronic clenbuterol treatment of WT mice increases glucose utilization in SKM in vivo.**

**Fig. 4: Chronic clenbuterol treatment decreases fatty acid oxidation in SKM in vivo.**

Given the central role of glucose in SKM metabolism and the outcome of our in vivo metabolic studies, we next closely examined metabolites in glucose-related pathways. In the fasted state, WT mice that had been treated with clenbuterol for 5 days showed significantly lower SKM glucose, pyruvate, lactate, fructose, and mannose levels (Fig. 3a, b), as compared to untreated WT mice, suggesting that clenbuterol treatment promoted the use of these metabolites as fuel source. When control and clenbuterol-treated mice were injected with an i.p. glucose bolus, the clenbuterol group showed lower blood glucose levels (215 ± 15 vs. 272 ± 14 mg/dl) and a significantly greater increase in SKM levels of glucose and pyruvate (Fig. 3c) and sugars such as fructose and mannose (Fig. 3d) 30 min after glucose injection, in agreement with increased glucose transport into SKM.

Interestingly, SKM GLUT1 protein levels and glucose-induced SKM GLUT4 translocation to the plasma membrane were not significantly different between the two groups of mice (Fig. 3e and Supplementary Fig. S7a–c), indicating that the ability of clenbuterol to alter SKM metabolism and improve glucose tolerance is not due to enhanced GLUT1 (total) or GLUT4 levels in the plasma membrane. Thus, the most likely scenario is that the clenbuterol-stimulated increase in glucose metabolism drives glucose uptake into SKM.

To further test this hypothesis, we measured the glycolysis rate in mice that had been treated with clenbuterol. We injected fasted lean WT mice with glucose containing a 3-³H-glucose tracer, collected plasma samples at multiple time points following the glucose bolus, and then determined the rate of ³H₂O production from 3-³H-glucose as a measure of glycolysis rate. Indeed, clenbuterol-treated mice showed a significantly higher glycolysis rate than control mice that had not received clenbuterol (Fig. 3f). These data strongly support the concept that clenbuterol leads to an increase in glucose utilization in SKM.

Moreover, SKM RNA-Seq data obtained from clenbuterol-treated WT mice showed an upregulation of several genes encoding glycolytic enzymes including Aldoa, Gapdh, Pgk1, and Eno1 (Fig. 3g, h), as compared to SKM from control mice that had not received clenbuterol. Further, the expression of Pdk1, Pdk2, and Pdk4, the kinases that phosphorylate and inhibit pyruvate dehydrogenase, the rate-limiting enzyme of glucose oxidation, was significantly decreased in SKM of clenbuterol-treated mice (Fig. 3g, h).

In addition, metabolomic analysis showed that SKM of fasted clenbuterol-treated mice displayed higher levels of glycogen breakdown intermediates and precursors, including maltotetraose and UDP-glucose (Fig. 3i). The clenbuterol-induced changes in the SKM levels of glycogen intermediates were accompanied by significantly lower expression levels of genes involved in the regulation of glycogen metabolism including Gsk3b, Gys1, and Gyg (Fig. 3j). Importantly, WT mice that had free access to food and were treated with clenbuterol showed a significant increase in SKM glycogen levels, as compared to control littermates that had not received clenbuterol (Fig. 3k). Consistent with the increased glycogen synthesis, mice that had been fasted for 24 h and then refed for 6 h showed significantly lower levels of phosphorylated GS (S641) in SKM (Fig. 3l).

In summary, the above data clearly indicate that chronic clenbuterol treatment leads to a metabolic reprogramming of SKM towards enhanced glucose utilization.

Clenbuterol treatment affects fatty acid oxidation in SKM

While glucose utilization was enhanced in SKM of WT mice treated with clenbuterol (Fig. 3), gene expression and metabolomics pathway analyses also suggested extensive changes in pathways involved in SKM fat oxidation (Fig. 4 and Supplementary Fig. 4b, c). Clenbuterol administration resulted in reduced SKM expression levels of genes coding for proteins involved in fatty acid uptake (Fabp3, Slc27a1, Cd36; Fig. 4b), lipolysis (Pnplap2; Fig. 4c), import of fatty acids into mitochondria (Acss1, Acsl1, Cpt1b, Cpt2; Fig. 4d), and β-oxidation (Acadm, Acadl, Acadvl, Hadh, Hadha, Hadhb, Acaa2, Eci1, Pccb, Crat, Acot2, Acot13; Fig. 4e). Metabolomic analysis indicated that clenbuterol-treated mice showed increased levels of SKM acylcarnitines (e.g., malonylcarnitine), as compared to control animals that had not received clenbuterol (Fig. 4f). Following clenbuterol treatment, we also observed changes in the levels of several classes of complex lipids including glycerophospholipids and ceramides, and in metabolites linked to phospholipid synthesis and turnover including phosphoethanolamine and glycerophosphocholine (Supplementary Data 1).

We further characterized clenbuterol-induced changes in SKM fatty acid metabolism using labeled palmitate metabolites. To directly measure fatty acid uptake into SKM, we injected mice with [9,10-³H]-(R)-2-bromopalmitate ([³H]-BROMO), a radioactive labeled analog of palmitate that is not a substrate for β-oxidation, but becomes trapped in slower metabolic processes of ω- and α-oxidation³⁷. We did not observe differences in [³H]-BROMO levels in SKM, liver, or adipose tissues of mice treated with clenbuterol water, as compared with mice consuming regular drinking water (Supplementary Fig. 8a). To determine whether the rate of β-oxidation was reduced in SKM of clenbuterol-treated mice, we injected overnight fasted mice with the uniformly labeled ¹³C stable isotope of palmitate ([U-¹³C]-palmitate, 50 μg/kg i.p.). We found that ¹³C enrichment in C₁₆-, C₁₄-, and C₁₂-acylcarnitines was stable at 25 min after [U-¹³C]-palmitate injection, and that similar enrichment levels were achieved in SKM of control mice, indicative of a pseudo isotopic steady state (Supplementary Fig. 8b, c). Interestingly, although there were no changes in ¹³C enrichment in SKM palmitate (Supplementary Fig. 8b), we detected significantly higher levels of ¹³C-labeled C₁₄-acylcarnitine in SKM of clenbuterol-treated mice (Supplementary Fig. 8c). No such changes were observed in the liver (Supplementary Fig. 8d, e). Since several genes within the β-oxidation pathway were downregulated in SKM following clenbuterol treatment (Fig. 4a, d, e), this observation supports the concept that clenbuterol treatment leads to a reduced rate of fatty acid oxidation in SKM.

To obtain additional information on the energy metabolism of mice maintained on clenbuterol drinking water, we subjected lean WT mice to indirect calorimetry measurements. After the recording of baseline parameters, mice were put on either clenbuterol or regular (vehicle) drinking water for 5 days (Supplementary Fig. 9a). As expected, after 5 days of clenbuterol treatment, mice showed significantly lower blood glucose levels (Supplementary Fig. 9b), as compared to mice maintained on regular drinking water. Clenbuterol administration did not cause any changes in food intake (Supplementary Fig. 9c) or locomotor activity (Supplementary Fig. 9d). However, we observed a slight increase in oxygen consumption (Supplementary Fig. 9e) and total energy expenditure (TEE; Supplementary Fig. 9f) in the clenbuterol-treated mice. More importantly, mice that received clenbuterol showed a significant increase in respiratory exchange ratio (RER; Supplementary Fig. 9g, h, j), specifically during the day/light period (Supplementary Fig. 9h) when mice are inactive. These results further corroborate that chronic clenbuterol treatment triggers a shift in SKM of preferential energy substrates from lipids to glucose, in agreement with the transcriptomic, metabolomic, and isotope labeling data (see above).

Improvements in glucose homeostasis following clenbuterol treatment are dependent on mTORC2 and AMPK signaling

To further investigate the cellular mechanisms underlying the beneficial metabolic effects of clenbuterol treatment, we performed western blotting studies based on the top regulated signaling pathways (Supplementary Fig. 4c), focusing on selected protein targets known to be involved in the regulation of glucose homeostasis in SKM. Lean WT mice that had been treated with vehicle or clenbuterol via the drinking water for 5 days were fasted overnight and then injected with saline or glucose. Quadriceps muscles were isolated 30 min later and processed for immunoblotting experiments. As previously observed in the refeeding experiment (Fig. 3l), clenbuterol treatment had a significant effect on the phosphorylation status of SKM glycogen synthase (GS) and the upstream kinase, GSK3β (Supplementary Fig. 10a–c). While pGS (S641) was significantly increased in saline-injected clenbuterol mice (fasting conditions), glucose treatment led to a significant (activating) dephosphorylation of GS in clenbuterol-treated mice only (Supplementary Fig. 10b). These data suggest that the observed improvements in glucose metabolism are potentially linked to enhanced glycogen metabolism, showing increases in glycogen breakdown during fasting (Fig. 3i) and enhanced glycogen storage upon glucose availability (Fig. 3k).

We also found that clenbuterol treatment decreased the phosphorylation of AKT (Supplementary Fig. 10d–f) and mammalian target of rapamycin (mTOR) (S2481, Supplementary Fig. 10i) in SKM tissue from WT mice. However, these changes were mostly driven by increased protein expression of total AKT (Supplementary Fig. 10h) and mTOR (Supplementary Fig. 10k), and not the amount of phosphorylated proteins per se (Supplementary Fig. 10g, j). Total AMPK was also slightly increased in SKM of clenbuterol-treated mice (Supplementary Fig. 10n). Interestingly, while a glucose bolus reduced AMPK phosphorylation in control animals (Supplementary Fig. 10a, l, m), pAMPK was already reduced in the clenbuterol group prior to glucose administration, and glucose treatment did not lead to a further reduction of the low pAMPK levels (Supplementary Fig. 10a, l, m).

Pathway analyses of differentially expressed genes following clenbuterol treatment (Supplementary Fig. 4c) showed enrichment of genes regulated by mTOR and AMPK. Indeed, previous in vitro studies demonstrated that isoproterenol, a non-subtype-selective β-AR agonist, could promote glucose uptake in the L6 muscle cell line in an mTORC2-dependent manner¹⁸, raising the possibility that mTORC2 may play a role in mediating the beneficial metabolic effects of SKM β₂-AR stimulation. To test this hypothesis, we carried out metabolic studies with mutant mice harboring an SKM-specific deletion of Rictor, a critical subunit of mTORC2 (SKM-Rictor-KO mice). We found that the improvements in glucose homeostasis caused by clenbuterol treatment were significantly reduced in SKM-Rictor-KO mice (Fig. 5a, b). On the other hand, treatment of WT mice with rapamycin (Supplementary Fig. 10o), for 24 h via the drinking water, 10 mg/l), an inhibitor of mTORC1, did not affect the improvement in glucose tolerance caused by clenbuterol treatment (Supplementary Fig. 10p, q). Moreover, clenbuterol treatment failed to increase SKM glycogen levels in the absence of SKM mTORC2 (Supplementary Fig. 10r).

**Fig. 5: Chronic clenbuterol treatment causes beneficial metabolic effects through SKM mTORC2 signaling.**

The importance of SKM mTORC2 signaling in mediating the β₂-AR-dependent beneficial metabolic effects was further examined by transcriptome analysis of clenbuterol-treated SKM-Rictor-KO mice, as compared to clenbuterol-treated control littermates. To identify genes that were regulated by clenbuterol in control mice, but not in SKM-Rictor-KO mice, a less stringent cut-off for the adjusted p-value (<0.1) was set for the initial analysis. SKM (gastrocnemius muscle) samples derived from control mice treated with clenbuterol showed 2639 differentially expressed genes (1336 upregulated, 1303 downregulated, adjusted p < 0.1), as compared to vehicle-treated mice (Fig. 5c). SKM samples from clenbuterol-treated SKM-Rictor-KO mice showed a similar number (2761) of differentially expressed genes (1398 upregulated, 1363 downregulated, adjusted p < 0.1), as compared to SKM samples from vehicle-treated SKM-Rictor-KO mice (Fig. 5c). Interestingly, there was an overlap of 1579 differentially expressed genes in these two data sets (Fig. 5c). Somewhat surprisingly, the clenbuterol-induced changes in gene expression of the major metabolite pathways (Supplementary Table 1) did not require the presence of SKM mTORC2, as clenbuterol caused similar alterations in gene expression profiles of SKM-Rictor-KO and control mice (Supplementary Table 1). However, we also identified many genes (407 and 683 (adjusted p < 0.05), respectively) that were differentially expressed only in SKM tissue of clenbuterol-treated control mice or clenbuterol-treated SKM-Rictor-KO mice, respectively (Fig. 5c). Among these genes, the perilipin 3 gene (Plin3) caught our particular attention, because Plin3 represents a regulator of lipid metabolism downstream of the mTORC2 complex³⁸. Previous work has shown that SKM-Rictor-KO mice shift to lipids as energy source by increasing Plin3 expression³⁸. Clenbuterol treatment significantly decreased Plin3 expression in SKM of control mice, but not in SKM-Rictor-KO mice, where SKM Plin3 expression was increased in the absence or presence of clenbuterol (Fig. 5d), providing a possible link between clenbuterol and mTORC2 in regulation of energy sources.

AMPK and mTORC2-dependent signaling pathways differentially regulate Plin3 expression³⁸. As the AMPK signaling pathway was among the significantly enriched pathways in SKM of clenbuterol-treated mice (Fig. 5e and Supplementary Fig. 4c) and SKM levels of endogenous AICAR and other adenosine derivatives were elevated (Supplementary Fig. 10s), we next investigated the potential role of SKM AMPK in mediating the beneficial metabolic effects of clenbuterol administration. For these experiments, we used transgenic mice that expressed a dominant-negative version of AMPK under the transcriptional control of the muscle-specific MCK promoter (MCK-AMPK-DN)³⁹. Remarkably, as observed with the SKM-Rictor-KO mice (Fig. 5a, b), the ability of clenbuterol treatment to improve glucose tolerance was nearly abolished in the MCK-AMPK-DN mice (Supplementary Fig. 10t, u).

In sum, these data clearly indicate that chronic clenbuterol treatment regulates SKM signaling via multiple metabolic sensors and signaling proteins, including β₂-AR, G_s, mTORC2, and AMPK.

Discussion

The present study has led to several important findings regarding the cellular and molecular mechanisms by which chronic clenbuterol treatment improves glucose homeostasis and other metabolic functions. We provide convincing evidence that the beneficial metabolic effects of chronic clenbuterol depend on the stimulation of SKM β₂-ARs, and that the coupling of these receptors to SKM G_s is essential for the manifestation of the clenbuterol-induced metabolic improvements. These conclusions are supported by studies using a newly developed mouse model (SKM-GsD mice) that allowed us to monitor the metabolic outcome of selective activation of SKM G_s signaling. In addition, comprehensive unbiased metabolomic and RNA-Seq studies provided important clues regarding the molecular mechanisms underlying the clenbuterol-induced improvements in SKM glucose homeostasis.

Specifically, we found that chronic clenbuterol treatment significantly enhanced glucose tolerance in lean and obese WT mice and the STZ model of β-cell dysfunction, without increasing plasma insulin levels or insulin tolerance (Fig. 1a–e). This effect was absent in SKM β₂-AR-KO and SKM-Gs-KO mice (Fig. 1g, h), indicating that the beneficial metabolic effects of systemic, chronic administration of the selective β₂-AR agonist are mediated by SKM β₂-ARs signaling via G_s. We previously showed that SKM-β-arrestins do not contribute to the beneficial metabolic effects caused by clenbuterol administration¹⁹. Although our study specifically focused on SKM, our findings also suggest that previously reported changes in mouse liver metabolism following prolonged treatment with clenbuterol⁴⁰ may be secondary to the action of clenbuterol at SKM β₂-AR.

The SKM-specific expression of a CNO-sensitive, GsD^{32,33,34,35,36} allowed us to study the in vivo metabolic consequences of selectively activating G_s in SKM in vivo. CNO treatment of SKM-GsD mice led to improved glucose tolerance (Fig. 2a, d and Supplementary Fig. S3g) by increasing glucose uptake into SKM in vivo (Fig. 2g). These findings mirror the effects observed after clenbuterol-induced activation of β₂-ARs in WT mice (Fig. 1). Taken together, these data further corroborate the central role of SKM β₂-AR/Gα_s signaling in meditating the metabolic effects caused by systemic administration of a β₂-AR agonist.

Chen et al.⁴¹ previously demonstrated that mice lacking Gα_s selectively in SKM display decreased glucose tolerance with no changes in insulin secretion or sensitivity. These data support our finding that activation of the β₂-AR/Gα_s pathway in SKM improves glucose homeostasis in an insulin-independent manner (Figs. 1b and 2b).

Previous work by the Lefkowitz lab has shown that both the β₁- and β₂-ARs can undergo PKA-dependent “G_s to G_i switching”^12,42. On the basis of these studies, we cannot completely rule out the possibility of a role for sequential signaling via G_s and G_i.

Surprisingly, the usual suspects in mediating improved glucose tolerance and glucose uptake in SKM, GLUT1, and GLUT4 did not show increased expression levels or enhanced glucose-induced translocation to the plasma membrane following clenbuterol treatment (Fig. 3e and Supplementary Fig. S7a–c). In contrast, previous in vitro studies suggested that β₂-AR stimulation leads to enhanced GLUT4 translocation in cultured muscle cells^18,20. These discrepant findings are most likely due to differences in experimental conditions. While the in vitro studies were performed with cultured cell lines overexpressing an epitope-tagged GLUT4 construct and short incubations with clenbuterol, the present study was carried out with isolated SKM prepared from WT mice treated with clenbuterol in vivo for a prolonged period of time and examined the translocation of endogenous GLUT4 following a glucose bolus.

Using unbiased transcriptomic and metabolomic approaches (Fig. 3 and Supplementary Fig. S4), we showed that clenbuterol treatment of WT mice caused a metabolic reprogramming, leading to enhanced glucose utilization in SKM. Although clenbuterol did not cause any changes in fat mass (Supplementary Fig. 2c), the expression levels of several key genes involved in fatty acid metabolism and oxidation, including carnitine palmitoyltransferase-1b (Cpt1b), were significantly downregulated in SKM following treatment with clenbuterol (Fig. 4a–e and Supplementary Table 1). These changes were accompanied by increased levels of acylcarnitines in SKM (Fig. 4f), further supporting the concept that chronic clenbuterol impairs fatty acid oxidation in SKM. This conclusion is also supported by the outcome of an experiment using a stable palmitate isotope (Supplementary Fig. 8b, c), as suggested by higher levels of C₁₄-acylcarnitines.

Decreased SKM oxidative capacity is often associated with insulin resistance². However, clenbuterol treatment did not affect insulin tolerance, but improved glucose tolerance with reduced insulin levels (Fig. 1a–e). The analysis of gene expression and functional data indicated that clenbuterol also increased the rate of glycolysis in SKM (Fig. 3a–c, f–h and Supplementary Fig. S9h), indicative of a shift in fuel utilization from fatty acid oxidation to increased glucose utilization to sustain SKM energy supply. Interestingly, mice lacking Cpt1b specifically in SKM show similar changes in glucose homeostasis as seen after clenbuterol treatment of WT mice, including impaired fatty acid oxidation⁴³, increased malonyl- and succinyl-carnitine levels, improved glucose tolerance, and enhanced basal glucose uptake in primary myotubes that is insulin-independent, indicative of a compensatory adaptation towards enhanced glucose usage⁴⁴. Moreover, the metabolic changes displayed by the SKM Cpt1b KO mice were dependent on increased signaling through the AMPK and mTORC2 pathways⁴⁴. In line with this observation, we demonstrated that inhibition of either of these two pathways interfered with the ability of clenbuterol to improve glucose tolerance (Fig. 5a, b and Supplementary Fig. S10t–u). In agreement with our findings, independent activation of either AMPK⁴⁵ or mTORC2⁴⁶ has been shown to increase SKM glycolysis rate. Furthermore, G_s signaling has been shown to activate AMPK under certain circumstances⁴⁷, which can interact with mTORC2 during energetic stress^48,49. These findings provide a possible link between enhanced SKM β₂-AR/G_s signaling and the increases in SKM AMPK and mTORC2 activity observed in the present study.

Somewhat surprisingly, the clenbuterol-induced changes in the expression of genes involved in major metabolic pathways did not require the presence of SKM mTORC2, as clenbuterol caused similar alterations in gene expression profiles in SKM-Rictor-KO and control mice (Supplementary Table 1). This observation suggests that SKM mTORC2 modifies SKM cellular functions primarily at the posttranscriptional level (following clenbuterol treatment) or in another manner that does not require changes at the transcriptional level. Thus, the precise mechanisms through which mTORC2 contributes to the beneficial metabolic effect of SKM β₂-AR stimulation requires more detailed future investigation.

Impaired glycogen synthesis in SKM is considered the earliest metabolic defect in the development of T2D². Interestingly, chronic clenbuterol treatment enhanced glycogen storage in SKM of freely fed mice (Fig. 3k), whereas fasted mice displayed increased levels of glycogen breakdown intermediates such as maltotetraose⁵⁰ and UDP-glucose (Fig. 3i), indicating that glycogen represents an important source of glucose as energy substrate under fasting conditions. We found that SKM β₂-AR stimulation regulated SKM glycogen metabolism both at the transcriptional and posttranslational level (through protein phosphorylation). Clenbuterol treatment decreased SKM gene expression levels of glycogenin (Gyg) and Gsk3b (Fig. 3j), two key regulators of glycogen synthesis. In agreement with these data, Gyg-deficient mice also showed increased glycogen levels in SKM and a switch to a more glycolysis-based fuel usage in SKM⁵¹. Similarly, SKM-specific GSK3β-KO mice display improved glucose tolerance and enhanced SKM glycogen deposition⁵². Moreover, consistent with our observation that clenbuterol treatment increased endogenous AICAR levels (Supplementary Fig. 10s) and required SKM AMPK to mediate its beneficial effects (Supplementary Fig. 10t–u), long-term activation of AMPK with AICAR led to increased glycogen accumulation in mouse or rat SKM^45,53.

Long-term treatment of human subjects with a β₂-AR agonist (terbutaline) led to an increase in non-oxidative disposal of glucose, e.g., in form of glycogen; however, the cellular mechanisms underlying this effect were not explored⁵⁴.

In the present study, clenbuterol treatment significantly affected the inhibitory phosphorylation of GS (pGS) (Supplementary Fig. 10a, b), based on glucose availability. In the fasted state (12 h, low blood glucose levels), clenbuterol administration increased SKM pGS levels (Supplementary Fig. 10b), consistent with a shift towards glycogen breakdown (Fig. 3i). In contrast, following glucose injection, SKM pGS levels significantly declined in clenbuterol-treated mice only (Supplementary Fig. 10a, b). A similar regulation of SKM pGS was observed when mice were refed after a 24 h-fasting period (Fig. 3l), indicative of the key role of SKM β₂-ARs in regulating SKM glycogen metabolism in a glucose/fuel-dependent manner. More detailed studies involving the infusion of stable glucose isotopes will be required to clearly define the fractions of glucose cycled via the glycogen and glycolysis pathways in SKM following clenbuterol treatment.

Although clenbuterol-mediated SKM hypertrophy was not the focus of this study, it is worth mentioning that the 5-day clenbuterol treatment led to a significant increase of several amino acids in SKM, following administration of a glucose bolus (Supplementary Fig. 6b). One possible explanation for this observation is that those mostly glucogenic amino acids are conserved for SKM protein synthesis in the presence of available glucose as a fuel source. However, the non-essential amino acids might also have been synthesized from glycolysis intermediates (Supplementary Fig. 6c, d). In agreement with this observation, it is known that glucose is rapidly converted into amino acids and other compounds/metabolites in SKM⁵⁵, and that glucose infusion significantly increases protein synthesis⁵⁶. As the clenbuterol-induced shift in preferential substrate utilization occurred in the absence of a significant increase in lean mass (Supplementary Fig. 2b), it is possible that the clenbuterol-mediated reprogramming of SKM towards enhanced glucose utilization also drives SKM hypertrophy that develops after clenbuterol treatment for several weeks¹⁶. Moreover, when fatty acid oxidation is impaired, amino acids can represent an important fuel source⁴³. Higher levels of N-acetylated amino acids (Supplementary Data 1), propionyl-carnitine (Fig. 4f), and succinyl-carnitine (Supplementary Fig. 5e) in clenbuterol-treated mice are potential indicators of increased amino acid catabolism/oxidation under fasting conditions.

A previous histological study reported that long-term β₂-AR stimulation promotes a slow-to-fast muscle fiber switch (oxidative-to-glycolytic)⁵⁷. Although our SKM RNA-Seq data did not reveal changes in classic muscle fiber markers like Myh7, Myh1, and Myh2, our unbiased metabolomic and transcriptomic approaches provided evidence for β₂-AR-mediated SKM metabolic reprogramming towards enhanced glucose utilization at both the transcriptional and metabolite level, consistent with the outcome of the study be Zeman et al.⁵⁷.

The β₂-AR is also abundantly expressed in human SKM (https://www.genecards.org/cgi-bin/carddisp.pl?gene=ADRB2), suggesting that clenbuterol may also cause beneficial effects on glucose homeostasis in humans. Clenbuterol and other β₂-AR agonists are well known for their therapeutic potential in treating muscle wasting and related SKM disorders¹⁶. Moreover, clenbuterol is used for the treatment of asthma and related pulmonary diseases in several European and Asian countries (http://drugapprovalsint.com/clenbuterol/), due to its ability to act on bronchial smooth muscle β₂-ARs. Kim et al.⁵⁸ recently reported that clenbuterol-induced SKM hypertrophy in mice requires SKM β-arrestin-1 signaling. As the beneficial effects of clenbuterol on glucose homeostasis are mediated by SKM G_s signaling, it should be possible to develop novel classes of β₂-AR agonists that stimulate SKM G_s but do not recruit β-arrestins. The data by Kim et al.⁵⁸ suggest that the potential use of such G protein-biased β₂-AR agonists for the treatment of SKM insulin resistance will not lead to the development of SKM hypertrophy.

In conclusion, by analyzing multiple new mouse models and using unbiased multiomic approaches, we provide clear evidence that systemic administration of a selective β₂-AR agonist (clenbuterol) significantly improves glucose homeostasis under physiological and pathophysiological conditions. We demonstrated that the metabolic improvements observed after a 5-day clenbuterol administration require the activation of the SKM β₂-AR/G_s complex and downstream AMPK and mTORC2 signaling. These signaling events eventually lead to a metabolic reprogramming of SKM towards enhanced glucose utilization. No other tissues or G protein signaling pathways appear to be involved in the clenbuterol-dependent metabolic improvements.

Our data strongly suggest that activation of G_s signaling in SKM (e.g., by the activation of G_s-coupled receptors endogenously expressed by SKM) or of components of downstream signaling pathways represents an attractive approach to develop novel classes of antidiabetic drugs targeted at modifying SKM metabolism.

Study limitations

Our study primarily focused on SKM phenotypes and did not explore the effect of systemic clenbuterol on other tissues expressing β₂-ARs. Although we clearly demonstrated that the beneficial metabolic effects seen after a 5-day clenbuterol treatment are dependent on SKM-β₂-ARs, we cannot completely exclude the possibility that the clenbuterol-induced changes in SKM (e.g., changes in gene transcription and metabolite levels) cause secondary changes in other tissues. The static metabolomic analyses that we performed provide a good overview of changes in SKM metabolite levels; however, infusion studies with isotope-labeled metabolite tracers are needed to draw clear conclusions about metabolite fluxes. Moreover, the precise molecular mechanisms through which chronic activation of SKM β₂-AR affects AMPK and mTORC2 signaling to alter SKM fuel utilization remain to be explored in future studies.

Methods

Materials

The sources of antibodies, chemicals, assay kits, and mouse lines used in this study are listed in Supplementary Table 2.

Mouse maintenance and diet

All mice were fed ad libitum and kept on a 12 h light, 12 h dark cycle at room temperature. Mice were maintained either on a standard mouse chow (7022 NIH-07 diet, 15% kcal fat, energy density 3.1 kcal/g, Envigo, Inc.) or a HFD (60% kcal from fat, energy density 5.49 kcal/g; # F3282, Bioserv) for at least 8 weeks.

All animal studies were carried out according to the US National Institutes of Health Guidelines for Animal Research and were approved by the NIDDK Institutional Animal Care and Use Committee.

Generation of SKM-specific KO and knock-in mice

To generate SKM-specific KO and knock-in mice, floxed mice (see Supplementary Table 2 for specific floxed lines) were crossed with HSA-Cre(ER^T2) mice⁵⁹. To avoid potential developmental changes, Cre recombinase activity was induced in 7- to 8-week-old HSA-Cre(ER^T2)-positive floxed/floxed mice by i.p. injection with tamoxifen (2 mg per day dissolved in corn oil) for 5 consecutive days. Tamoxifen-injected Cre-negative floxed/floxed littermates served as control mice.

In vivo metabolic studies

Unless stated otherwise, all metabolic tests were performed on male littermates (age range: 10–30 weeks) using standard protocols. For i.p. GTTs (ipGTT), mice were fasted overnight for 15 h and blood glucose levels were measured before (0 min) and at defined time points after i.p. injection of normal saline containing glucose (2 g/kg for mice consuming normal chow; 1 g/kg for mice on HFD). For ITTs, mice were fasted for 4 h and blood glucose levels were measured before (0 min) and at indicated time points after i.p. injection of human insulin (0.75 IU/kg or 1 IU/kg, as indicated; Humulin R, Eli Lilly). Blood glucose levels were determined using a manual blood glucose meter (Contour; Bayer). To study GSIS, mice were fasted overnight for 15 h and blood samples were collected in heparinized capillary tubes (Fisher Scientific) before (0 min) and 5, 15, and 30 min following the i.p. injection of glucose (2 g/kg or 1 g/kg, as indicated). Samples were centrifuged (5000 × g, 10 min, 4 °C) for plasma collection and plasma insulin levels were determined using an ultra-sensitive mouse insulin ELISA kit (Crystal Chem, Inc.).

Clenbuterol administration

For chronic clenbuterol treatment studies, WT mice consumed drinking water containing clenbuterol (30 mg/l) or regular drinking water for 5 days prior to metabolic experiments or tissue collection. During this 5-day period, mice consumed 3.5 ± 0.06 ml of clenbuterol water per day, resulting in an average clenbuterol dose of 104.7 ± 1.2 μg per mouse per day. For chronic clenbuterol studies performed with transgenic mice, baseline ipGTTs were performed with control and the indicated KO mice as described above. Two days later, both control and mutant mice started to consume clenbuterol drinking water. After 5 days on clenbuterol water, mice were subjected to another ipGTT.

CNO administration

For long-term stimulation of G_s signaling in SKM, control and SKM-GsD mice received CNO continuously for 7 days by mixing CNO into the drinking water at a concentration of 250 mg/l, as described previously⁸.

STZ model

To induce β-cell dysfunction, STZ treatment protocol has been used²⁸, which has been previously shown to destroy about 70–80% of β-cells. Specifically, lean WT mice were fasted for 5 h and injected with a relatively low dose (50 mg/kg i.p.) of STZ for 5 consecutive days. Metabolic studies were initiated seven days after the last STZ injection.

Rapamycin administration

To investigate whether activation of the mTORC1 complex contributes to the metabolic effects of long-term clenbuterol treatment, rapamycin (10 mg/l) or vehicle was provided for the initial 24 h of a 36 h treatment with clenbuterol drinking water. These experimental conditions were chosen to selectively inhibit the mTORC1 complex^60,61 (see Supplementary Fig. 10o for a scheme of the experimental design).

Body composition analysis

Mouse body mass composition (lean and fat mass) was determined using a 3-in-1 EchoMRI Analyzer (Echo Medical System).

Indirect calorimetry measurements

TEE, RER (O₂ consumed/CO₂ produced), food intake, and locomotor activity (assayed by beam breaks) were measured simultaneously in mice housed at 22 °C using an Oxymax/CLAMS (Columbus Instruments). Sampling was performed every 13 min, measuring from 12 chambers. Mice were adapted in the chambers for 2 days and then baseline data were collected for 3 days. Water and food were provided ad libitum during the sampling period. For chronic clenbuterol studies, mice consumed clenbuterol (30 mg/l) or regular drinking water for 5 days. Treatment data were recorded for the last 3 days of clenbuterol treatment (see Supplementary Fig. 9a for a scheme of the experimental design). Data are presented as average parameters per day for the recorded period.

In vivo [¹⁴C]2-deoxyglucose uptake

To measure glucose uptake into individual tissues in vivo, mice were fasted overnight for 14–16 h and then injected i.p. with saline containing 2 g/kg glucose and 10 μCi of [¹⁴C]2-deoxyglucose ([¹⁴C]2-DG) (Perkin Elmer). Mice were killed 2 h later, and SKM and other tissues were collected. The tissue content of [¹⁴C]2-DG-6-phosphate was determined as a measure of SKM glucose uptake, as described previously⁶².

Glycolysis rate determination

Overnight (15 h) fasted mice were injected with glucose (2 g/kg i.p.) containing 2.5 mCi/kg [3-³H]-glucose. Blood samples were collected from the tail vein before and 5, 10, 15, 30, 45, and 60 min post injection. Plasma samples were processed as described previously and glycolysis rate was estimated as the rate of ³H₂O appearance⁶³.

Glycogen measurements

Glycogen content in SKM was determined using a glycogen assay kit (Cayman Chemical), according to the manufacturer’s instructions.

In vivo GLUT4 translocation

WT mice consumed clenbuterol (30 mg/l) or regular drinking water for 5 days. Mice were then fasted overnight (15 h) and injected i.p. with glucose (2 g/kg). Quadriceps muscles were isolated 15 min after the glucose bolus, mounted in Tissue-Tek® medium, frozen in liquid nitrogen-cooled isopentane, and cryo-sectioned (7 μm) using a Leica CM3050S cryostat (chamber and object temperature was set to −22 °C). Sections were attached to glass slides and fixed for 10 min in ice-cold 4% paraformaldehyde in 0.1 M Sorensen’s phosphate buffer (pH 7.3), washed 3 × 10 min with 1× phosphate-buffered saline (PBS), and then incubated with a rabbit polyclonal antibody against GLUT4 (Thermo Scientific, PA5-23052; antibody was diluted in 1× PBS to 10 μg/ml; overnight incubation at 4 °C). Sections were washed 3 × 10 min and then incubated for 1 h with a goat anti-rabbit F(ab’)₂ fragment-specific antibody conjugated to Alexa-594 (Jackson ImmunoResearch, 111-585-047; antibody dilution: 3.75 μg/ml in 1× PBS). Sections were washed 3 × 10 min in 1× PBS and incubated for 15 min with wheat germ agglutinin (WGA) conjugated to Alexa-488 diluted to 5 μg/ml in 1× PBS, followed by staining for 5 min with Hoechst 33342 diluted in 1× PBS to 2 μg/ml. Confocal images were taken using a Nikon A1R microscope and an Apo TIRF × 60/1.49 oil differential interference contrast (DIC) objective. To quantify GLUT4 expression on the cell surface, five images were analyzed per mouse. In each image, 25 membrane areas were randomly selected and the GLUT4 signal was quantified in the area positive for WGA staining. The average GLUT4 signal for each mouse was calculated.

Quantitative gene expression analysis

Tissues were collected and homogenized in TRIzol (Thermo Fisher Scientific). Total RNA was isolated using the RNeasy Mini Kit (Qiagen) and RNA quantity was measured with a spectrophotometer (Nanodrop ND 1000; NanoDrop Products, Wilmington, DE). For qRT-PCR studies, 1 mg of total RNA was reversely transcribed (SuperScript III Reverse Transcriptase, Invitrogen) using oligo(dT) primers. qRT-PCR was performed using SYBR Green Master Mix (Applied Biosystems) according to the manufacturer’s instructions. Data were normalized to the expression of β₂-microglobulin.

RNA-Seq studies

For chronic clenbuterol studies, lean WT mice (12-week-old males) consumed clenbuterol (30 mg/l) or regular drinking water for 5 days. Subsequently, quadriceps muscles were isolated from overnight (15 h) fasted or freely fed mice. Control and SKM-Rictor-KO mice were treated in the same fashion, but gastrocnemius muscle samples were collected from fed mice only. Total RNA was prepared from frozen tissues as described above. The RNA quality of all samples was analyzed on the Agilent 2100 bioanalyzer using the RNA 6000 Nano Chip. cDNA libraries were generated using New England Biolabs Ultra II kit following the manufacturer’s instructions. Indexed libraries of good quality (RNA Integrity Number > 8) were pooled and used for sequencing on a HiSeq 2500 Illumina Sequencing System. Single end 50 bp reads were mapped to mouse genome mm10. Analysis of differentially expressed genes was performed on the Genomatix Genome Analyzer using the DESeq2 (two-tailed Wald’s test) software package. Functional enrichment and pathway analysis of differentially expressed genes was performed using Qiagen IPA software and ToppGene Suite⁶⁴.

Metabolomics

WT mice (10-week-old males) consumed clenbuterol (30 mg/l) or regular drinking water for 5 days. Quadriceps muscles were then collected and freeze-clamped from mice that had been fasted overnight (15 h). In addition, overnight (15 h) fasted clenbuterol and control WT mice were injected with glucose (2 g/kg i.p.) and quadriceps muscles were isolated and freeze-clamped 30 or 60 min after the i.p. glucose bolus. Sample preparation and analysis was carried out at Metabolon, Inc. (Durham, NC). In brief, sample preparation involved protein precipitation and removal with methanol, shaking, and centrifugation. The resulting extracts were profiled on an accurate mass global metabolomics platform consisting of multiple arms differing by chromatography methods and mass spectrometry ionization modes to achieve broad coverage of compounds differing by physiochemical properties such as mass, charge, chromatographic separation, and ionization behavior. The details of this platform have been described previously⁶⁵. Metabolites were identified by automated comparison of the ion features in the experimental samples to a reference library of chemical standard entries that included retention time, molecular weight (m/z), preferred adducts, and in-source fragments, as well as associated MS spectra, and were curated by visual inspection for quality control using software developed at Metabolon^66,67.

Statistical analysis was performed using two-way analysis of variance (ANOVA) contrasts, main and interaction effect tests as standard statistical methods used by Metabolon⁶⁸.

[³H]-BROMO uptake studies

In vivo fatty acid uptake was examined in WT male mice treated with clenbuterol (30 mg/l) or regular drinking water for 5 days. Mice were fasted overnight (15 h) and injected i.p. with 200 μl of olive oil containing 2 μCi of (R)-2-bromopalmitic acid [9,10-³H] ([³H]-BROMO), a partially metabolizable long-chain fatty acid tracer (American Radiolabeled Chemicals, St. Louis, MO). Tissues (~150 mg) were collected 1 h later and solubilized in 1 ml of Biosol (National Diagnostics, Charlotte, NC) for 3 h in a 50 °C water bath, followed by another 1 h incubation in the presence of 0.3 ml 30% hydrogen peroxide. Samples were mixed with 10 ml of scintillation solution (Bioscint, National Diagnostics, Charlotte, NC) and counted using a Tri-Carb 2910 TR liquid scintillation analyzer (Perkin Elmer, Waltham, MA). Data were normalized to mg of tissue.

Stable isotope ([U-¹³C]-palmitate) studies

Lean WT mice (12-week-old males) consumed clenbuterol water (30 mg/l) or regular drinking water for 5 days. On the day of the experiment, overnight (15 h) fasted mice were injected with [U-¹³C]-palmitate (50 μg/kg i.p.). The injection solution was prepared as follows: [U-¹³C]-palmitate powder was dissolved in 50% ethanol and further diluted in sterile 0.9% saline containing bovine serum albumin (BSA) to the final concentration (2.5 mg/ml [U-¹³C]-palmitate, 5% ethanol, 10% BSA). BSA coupling of palmitate was achieved by shaking the incubation solution overnight at 37 °C. Mice were killed 25 min after the injection and isolated tissues were snap-frozen in liquid nitrogen for metabolite extraction.

Acylcarnitine and stable isotope enrichment UPLC-Quadrupole Time of Flight Mass Spectrometer (QTOFMS) analysis

Quadriceps muscles were homogenized in 14 µl/mg tissue of 3 : 4 water : methanol using a Precellys tissue homogenizer (setting: shaking at 6500 r.p.m. twice for 30 s). Chloroform containing 0.5 µM C17 ceramide (d18:1/17:0, Avanti Polar Lipids) was added to each sample at a ratio of 16 µl/mg tissue. The organic layer was transferred to a glass tube and dried under a gentle stream of nitrogen. Samples were reconstituted in isopropanol/methanol/chloroform (4/2/1) and 5 μl was injected on to a Waters ACQUITY ultra-performance liquid chromatography (UPLC) CSH C18 1.7 μm column (2.1 × 100 mm) maintained at 55 °C. The mobile phase, flow rate, and gradient conditions were as previously described⁶⁹. UPLC-QTOFMS analysis was performed in a Waters SYNAPT G2-Si in positive and negative electrospray ionization modes. Data were analyzed using Targetlynx XS and the percentage of neutral isotope was calculated as a peak area ratio of complete ¹³C-labeled metabolite/¹²C-labeled metabolite × 100%.

Western blotting experiments

Tissues were isolated quickly, frozen in liquid nitrogen, and stored at −80 °C until use. For western blotting studies, frozen tissues were homogenized in ice-cold RIPA buffer (Sigma Aldrich) and protein concentrations were determined using a BCA protein assay (Thermo Fisher Scientific). Protein extracts were separated on NuPAGE 4–12% Bis-Tris or, for high molecular mass protein targets, on 3–8% Tris-Acetate gels (Thermo Fisher Scientific) and blotted onto nitrocellulose membranes (Bio-Rad). Membranes were blocked for 1 h at room temperature in TBS-T (0.1%) containing 5% BSA. Membranes were then incubated overnight with primary antibodies at 4 °C. Following three washing steps in TBS-T (0.1%), membranes were incubated with horseradish peroxidase-conjugated secondary antibodies for 1 h at room temperature. After thorough washing, proteins were visualized with SuperSignal West Dura Extended Duration Substrate (Thermo Fisher Scientific) on the c600 Imaging System (Azure Biosystems). Immunoreactive bands were quantified using Image J Software (NIH). Uncropped images are provided in the Source Data file.

Statistics

Data are expressed as mean ± SEM for the indicated number of observations. Data were assessed for statistical significance by two-way ANOVA tests, followed by the indicated post hoc tests, or by using a two-tailed unpaired Student’s t-test, as appropriate. A p-value of <0.05 was considered statistically significant. The specific statistical tests that were used are indicated in the figure legends. Precise p-values are provided in the Source Data File.

Reporting summary

Further information on research design is available in the Nature Research Reporting Summary linked to this article.

Data availability

Source data are provided as a Source Data file. Levels of all by Metabolon detected metabolites are provided as Supplementary Data 1 and raw data can be downloaded from MetaboLights under https://www.ebi.ac.uk/metabolights/MTBLS467 (study number: MTBLS467). The raw RNA-seq data can be downloaded from the NCBI Sequence Read Archive under reference number RNA seq-PRJNA756816 [https://www.ncbi.nlm.nih.gov/bioproject/PRJNA756816]. Source data are provided with this paper.

References

Sola, D. et al. Sulfonylureas and their use in clinical practice. Arch. Med. Sci. 11, 840–848 (2015).
Article CAS PubMed PubMed Central Google Scholar
DeFronzo, R. A. & Tripathy, D. Skeletal muscle insulin resistance is the primary defect in type 2 diabetes. Diabetes Care 32, S157–S163 (2009).
Article CAS PubMed PubMed Central Google Scholar
Sriram, K. & Insel, P. A. G protein-coupled receptors as targets for approved drugs: how many targets and how many drugs? Mol. Pharm. 93, 251–258 (2018).
Article CAS Google Scholar
Mortazavi, A., Williams, B. A., McCue, K., Schaeffer, L. & Wold, B. Mapping and quantifying mammalian transcriptomes by RNA-Seq. Nat. Methods 5, 621–628 (2008).
Article CAS PubMed Google Scholar
Hutchinson, D. S. & Bengtsson, T. AMP-activated protein kinase activation by adrenoceptors in L6 skeletal muscle cells: mediation by alpha1-adrenoceptors causing glucose uptake. Diabetes 55, 682–690 (2006).
Article CAS PubMed Google Scholar
Horinouchi, T. et al. Endothelin-1 suppresses insulin-stimulated Akt phosphorylation and glucose uptake via GPCR kinase 2 in skeletal muscle cells. Br. J. Pharm. 173, 1018–1032 (2016).
Article CAS Google Scholar
Merlin, J. et al. The M3-muscarinic acetylcholine receptor stimulates glucose uptake in L6 skeletal muscle cells by a CaMKK-AMPK-dependent mechanism. Cell Signal 22, 1104–1113 (2010).
Article CAS PubMed Google Scholar
Bone, D. B. J. et al. Skeletal muscle-specific activation of Gq signaling maintains glucose homeostasis. Diabetes, https://doi.org/10.2337/db18-0796 (2019).
Lefkowitz, R. J., Stadel, J. M. & Caron, M. G. Adenylate cyclase-coupled beta-adrenergic receptors: structure and mechanisms of activation and desensitization. Annu. Rev. Biochem. 52, 159–186 (1983).
Article CAS PubMed Google Scholar
Li, F., De Godoy, M. & Rattan, S. Role of adenylate and guanylate cyclases in beta1-, beta2-, and beta3-adrenoceptor-mediated relaxation of internal anal sphincter smooth muscle. J. Pharm. Exp. Ther. 308, 1111–1120 (2004).
Article CAS Google Scholar
Xiao, R. P. Beta-adrenergic signaling in the heart: dual coupling of the beta2-adrenergic receptor to G(s) and G(i) proteins. Sci. STKE 2001, re15 (2001).
Article CAS PubMed Google Scholar
Daaka, Y., Luttrell, L. M. & Lefkowitz, R. J. Switching of the coupling of the beta2-adrenergic receptor to different G proteins by protein kinase A. Nature 390, 88–91 (1997).
Article CAS PubMed ADS Google Scholar
Carr, R. 3rd et al. β-Arrestin-biased signaling through the β2-adrenergic receptor promotes cardiomyocyte contraction. Proc. Natl Acad. Sci. USA 113, E4107–E4116 (2016).
Article PubMed PubMed Central Google Scholar
Luttrell, L. M. & Lefkowitz, R. J. The role of beta-arrestins in the termination and transduction of G-protein-coupled receptor signals. J. Cell Sci. 115, 455–465 (2002).
Article CAS PubMed Google Scholar
Pakharukova, N., Masoudi, A., Pani, B., Staus, D. P. & Lefkowitz, R. J. Allosteric activation of proto-oncogene kinase Src by GPCR-beta-arrestin complexes. J. Biol. Chem., https://doi.org/10.1074/jbc.RA120.015400 (2020).
Lynch, G. S. & Ryall, J. G. Role of beta-adrenoceptor signaling in skeletal muscle: implications for muscle wasting and disease. Physiol. Rev. 88, 729–767 (2008).
Article CAS PubMed Google Scholar
Jessen, S. et al. Hypertrophic effect of inhaled beta(2) -agonist with and without concurrent exercise training: a randomized controlled trial. Scand. J. Med. Sci. Sports 28, 2114–2122 (2018).
Article CAS PubMed Google Scholar
Sato, M. et al. Improving type 2 diabetes through a distinct adrenergic signaling pathway involving mTORC2 that mediates glucose uptake in skeletal muscle. Diabetes 63, 4115–4129 (2014).
Article CAS PubMed Google Scholar
Meister, J. et al. Metabolic effects of skeletal muscle-specific deletion of beta-arrestin-1 and -2 in mice. PLoS Genet. 15, e1008424 (2019).
Article CAS PubMed PubMed Central Google Scholar
Kalinovich, A. et al. Treatment with a beta-2-adrenoceptor agonist stimulates glucose uptake in skeletal muscle and improves glucose homeostasis, insulin resistance and hepatic steatosis in mice with diet-induced obesity. Diabetologia. https://doi.org/10.1007/s00125-020-05171-y (2020).
Philipson, L. H. beta-Agonists and metabolism. J. Allergy Clin. Immunol. 110, S313–S317 (2002).
Article CAS PubMed Google Scholar
Regard, J. B., Sato, I. T. & Coughlin, S. R. Anatomical profiling of G protein-coupled receptor expression. Cell 135, 561–571 (2008).
Article CAS PubMed PubMed Central Google Scholar
Jensen, J., Aslesen, R., Ivy, J. L. & Brors, O. Role of glycogen concentration and epinephrine on glucose uptake in rat epitrochlearis muscle. Am. J. Physiol. 272, E649–E655 (1997).
CAS PubMed Google Scholar
Ngala, R. A. et al. Beta2-adrenoceptors and non-beta-adrenoceptors mediate effects of BRL37344 and clenbuterol on glucose uptake in soleus muscle: studies using knockout mice. Br. J. Pharm. 158, 1676–1682 (2009).
Article CAS Google Scholar
Ngala, R. A. et al. Metabolic responses to BRL37344 and clenbuterol in soleus muscle and C2C12 cells via different atypical pharmacologies and beta2-adrenoceptor mechanisms. Br. J. Pharm. 155, 395–406 (2008).
Article CAS Google Scholar
Liu, Y. L., Cawthorne, M. A. & Stock, M. J. Biphasic effects of the beta-adrenoceptor agonist, BRL 37344, on glucose utilization in rat isolated skeletal muscle. Br. J. Pharm. 117, 1355–1361 (1996).
Article CAS Google Scholar
Richter, E. A., Ruderman, N. B. & Galbo, H. Alpha and beta adrenergic effects on metabolism in contracting, perfused muscle. Acta Physiol. Scand. 116, 215–222 (1982).
Article CAS PubMed Google Scholar
Jain, S. et al. Chronic activation of a designer G(q)-coupled receptor improves beta cell function. J. Clin. Invest. 123, 1750–1762 (2013).
Article CAS PubMed PubMed Central Google Scholar
Andre, C. et al. Transgenic mice carrying the human beta 2-adrenergic receptor gene with its own promoter overexpress beta 2-adrenergic receptors in liver. Eur. J. Biochem. 241, 417–424 (1996).
Article CAS PubMed Google Scholar
Rubenstein, A. B. et al. Single-cell transcriptional profiles in human skeletal muscle. Sci. Rep. 10, 229 (2020).
Article CAS PubMed PubMed Central ADS Google Scholar
Wang, L. et al. Use of DREADD technology to identify novel targets for antidiabetic drugs. Annu. Rev. Pharmacol. Toxicol. https://doi.org/10.1146/annurev-pharmtox-030220-121042 (2020).
Guettier, J. M. et al. A chemical-genetic approach to study G protein regulation of beta cell function in vivo. Proc. Natl Acad. Sci. USA 106, 19197–19202 (2009).
Article CAS PubMed PubMed Central ADS Google Scholar
Inoue, A. et al. Illuminating G-protein-coupling selectivity of GPCRs. Cell 177, 1933–1947.e1925 (2019).
Article CAS PubMed PubMed Central Google Scholar
Akhmedov, D. et al. Gs-DREADD knock-in mice for tissue-specific, temporal stimulation of cAMP signaling. Mol. Cellular Biol. https://doi.org/10.1128/mcb.00584-16 (2017).
Wang, L. et al. Selective activation of Gs signaling in adipocytes causes striking metabolic improvements in mice. Mol. Metab. https://doi.org/10.1016/j.molmet.2019.06.018 (2019).
Caron, A. et al. Adipocyte Gs but not Gi signaling regulates whole-body glucose homeostasis. Mol. Metab. https://doi.org/10.1016/j.molmet.2019.06.019 (2019).
Shearer, J. et al. Long chain fatty acid uptake in vivo: comparison of [125I]-BMIPP and [3H]-bromopalmitate. Lipids 43, 703–711 (2008).
Article CAS PubMed PubMed Central Google Scholar
Kleinert, M. et al. mTORC2 and AMPK differentially regulate muscle triglyceride content via Perilipin 3. Mol. Metab. 5, 646–655 (2016).
Article CAS PubMed PubMed Central Google Scholar
Mu, J., Brozinick, J. T. Jr., Valladares, O., Bucan, M. & Birnbaum, M. J. A role for AMP-activated protein kinase in contraction- and hypoxia-regulated glucose transport in skeletal muscle. Mol. Cell 7, 1085–1094 (2001).
Article CAS PubMed Google Scholar
Kalinovich, A. et al. Treatment with a beta-2-adrenoceptor agonist stimulates glucose uptake in skeletal muscle and improves glucose homeostasis, insulin resistance and hepatic steatosis in mice with diet-induced obesity. Diabetologia 63, 1603–1615 (2020).
Article CAS PubMed PubMed Central Google Scholar
Chen, M. et al. G(s)alpha deficiency in skeletal muscle leads to reduced muscle mass, fiber-type switching, and glucose intolerance without insulin resistance or deficiency. Am. J. Physiol. Cell Physiol. 296, C930–C940 (2009).
Article CAS PubMed PubMed Central Google Scholar
Martin, N. P., Whalen, E. J., Zamah, M. A., Pierce, K. L. & Lefkowitz, R. J. PKA-mediated phosphorylation of the beta1-adrenergic receptor promotes Gs/Gi switching. Cell. Signal. 16, 1397–1403 (2004).
Article CAS PubMed Google Scholar
Wicks, S. E. et al. Impaired mitochondrial fat oxidation induces adaptive remodeling of muscle metabolism. Proc. Natl Acad. Sci. USA 112, E3300–E3309 (2015).
Article CAS PubMed PubMed Central Google Scholar
Vandanmagsar, B. et al. Impaired mitochondrial fat oxidation induces FGF21 in muscle. Cell Rep. 15, 1686–1699 (2016).
Article CAS PubMed PubMed Central Google Scholar
Hunter, R. W., Treebak, J. T., Wojtaszewski, J. F. & Sakamoto, K. Molecular mechanism by which AMP-activated protein kinase activation promotes glycogen accumulation in muscle. Diabetes 60, 766–774 (2011).
Article CAS PubMed PubMed Central Google Scholar
Kleinert, M. et al. Acute mTOR inhibition induces insulin resistance and alters substrate utilization in vivo. Mol. Metab. 3, 630–641 (2014).
Article CAS PubMed PubMed Central Google Scholar
Hutchinson, D. S., Summers, R. J. & Bengtsson, T. Regulation of AMP-activated protein kinase activity by G-protein coupled receptors: potential utility in treatment of diabetes and heart disease. Pharm. Ther. 119, 291–310 (2008).
Article CAS Google Scholar
Fu, W. & Hall, M. N. Regulation of mTORC2 signaling. Genes (Basel) 11, https://doi.org/10.3390/genes11091045 (2020).
Kazyken, D. et al. AMPK directly activates mTORC2 to promote cell survival during acute energetic stress. Sci. Signal. 12, https://doi.org/10.1126/scisignal.aav3249 (2019).
Olavarria, J. M. The metabolism of oligosaccharides. J. Biol. Chem. 235, 3058–3060 (1960).
Article CAS PubMed Google Scholar
Testoni, G. et al. Lack of glycogenin causes glycogen accumulation and muscle function impairment. Cell Metab. 26, 256–266 e254 (2017).
Article CAS PubMed Google Scholar
Patel, S. et al. Tissue-specific role of glycogen synthase kinase 3beta in glucose homeostasis and insulin action. Mol. Cell Biol. 28, 6314–6328 (2008).
Article CAS PubMed PubMed Central Google Scholar
Holmes, B. F., Kurth-Kraczek, E. J. & Winder, W. W. Chronic activation of 5’-AMP-activated protein kinase increases GLUT-4, hexokinase, and glycogen in muscle. J. Appl. Physiol. 87, 1990–1995 (1999). (1985).
Article CAS PubMed Google Scholar
Scheidegger, K., Robbins, D. C. & Danforth, E. Jr. Effects of chronic beta receptor stimulation on glucose metabolism. Diabetes 33, 1144–1149 (1984).
Article CAS PubMed Google Scholar
Vrba, R., Gaitonde, M. K. & Richter, D. The conversion of glucose carbon into protein in the brain and other organs of the rat. J. Neurochem. 9, 465–475 (1962).
Article CAS PubMed Google Scholar
David, M. & Avi-Dor, Y. Stimulation of protein synthesis in cultured heart muscle cells by glucose. Biochem. J. 150, 405–411 (1975).
Article CAS PubMed PubMed Central Google Scholar
Zeman, R. J., Ludemann, R., Easton, T. G. & Etlinger, J. D. Slow to fast alterations in skeletal muscle fibers caused by clenbuterol, a beta 2-receptor agonist. Am. J. Physiol. 254, E726–E732 (1988).
CAS PubMed Google Scholar
Kim, J. et al. beta-arrestin 1 regulates beta2-adrenergic receptor-mediated skeletal muscle hypertrophy and contractility. Skelet. Muscle 8, 39 (2018).
Article CAS PubMed PubMed Central Google Scholar
Schuler, M., Ali, F., Metzger, E., Chambon, P. & Metzger, D. Temporally controlled targeted somatic mutagenesis in skeletal muscles of the mouse. Genesis 41, 165–170 (2005).
Article CAS PubMed Google Scholar
Eghtesad, S., Jhunjhunwala, S., Little, S. R. & Clemens, P. R. Rapamycin ameliorates dystrophic phenotype in mdx mouse skeletal muscle. Mol. Med. 17, 917–924 (2011).
Article CAS PubMed PubMed Central Google Scholar
Schreiber, K. H. et al. Rapamycin-mediated mTORC2 inhibition is determined by the relative expression of FK506-binding proteins. Aging Cell 14, 265–273 (2015).
Article CAS PubMed PubMed Central Google Scholar
Li, Y. Q. et al. Gsalpha deficiency in adipose tissue improves glucose metabolism and insulin sensitivity without an effect on body weight. Proc. Natl Acad. Sci. USA 113, 446–451 (2016).
Article CAS PubMed ADS Google Scholar
Ayala, J. E., Bracy, D. P., McGuinness, O. P. & Wasserman, D. H. Considerations in the design of hyperinsulinemic-euglycemic clamps in the conscious mouse. Diabetes 55, 390–397 (2006).
Article CAS PubMed Google Scholar
Chen, J., Bardes, E. E., Aronow, B. J. & Jegga, A. G. ToppGene Suite for gene list enrichment analysis and candidate gene prioritization. Nucleic Acids Res. 37, W305–W311 (2009).
Article CAS PubMed PubMed Central Google Scholar
Ford, L. et al. Precision of a clinical metabolomics profiling platform for use in the identification of inborn errors of metabolism. J. Appl. Lab. Med. 5, 342–356 (2020).
Article PubMed Google Scholar
Dehaven, C. D., Evans, A. M., Dai, H. & Lawton, K. A. Organization of GC/MS and LC/MS metabolomics data into chemical libraries. J. Cheminform. 2, 9 (2010).
Article PubMed PubMed Central Google Scholar
Evans, A. M., DeHaven, C. D., Barrett, T., Mitchell, M. & Milgram, E. Integrated, nontargeted ultrahigh performance liquid chromatography/electrospray ionization tandem mass spectrometry platform for the identification and relative quantification of the small-molecule complement of biological systems. Anal. Chem. 81, 6656–6667 (2009).
Article CAS PubMed Google Scholar
Storey, J. D. & Tibshirani, R. Statistical significance for genomewide studies. Proc. Natl Acad. Sci. USA 100, 9440–9445 (2003).
Article MathSciNet CAS PubMed PubMed Central MATH ADS Google Scholar
Brocker, C. N. et al. Extrahepatic PPARalpha modulates fatty acid oxidation and attenuates fasting-induced hepatosteatosis in mice. J. Lipid Res. 59, 2140–2152 (2018).
Article CAS PubMed PubMed Central Google Scholar

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Acknowledgements

This research was funded by the Intramural Research Program of the National Institute of Diabetes and Digestive and Kidney Diseases (NIDDK, NIH). We thank Dr. Daniel Metzger (Université de Strasbourg, Illkirch, France) for providing the HSA-Cre(ER^T2) mice; Yinyan Ma and Naili Liu (Mouse Metabolism Core, NIDDK) for technical assistance in some of the metabolic studies; Dr. Harold Smith and several of his coworkers (NIDDK Genomics Core) for their help with the RNA-seq work. We thank Kristopher W. Krausz (NCI, NIH) for assistance with the mass spectrometry studies and Dr. Frank J. Gonzalez (NCI, NIH) for helpful advice and support of this work. Dr. Markus Rüegg (University of Basel) generously provided the SKM-specific Rictor KO founder mice.

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These authors contributed equally: Jaroslawna Meister, Derek B. J. Bone.

Authors and Affiliations

Molecular Signaling Section, Laboratory of Bioorganic Chemistry, National Institute of Diabetes and Digestive and Kidney Diseases, Bethesda, MD, 20892, USA
Jaroslawna Meister, Derek B. J. Bone, Luiz F. Barella, Regina J. Lee, Amanda H. Cohen, Yinghong Cui & Jürgen Wess
Departments of Nutrition, Exercise and Sports, University of Copenhagen, København, Denmark
Jonas R. Knudsen, Maximilian Kleinert, Thomas E. Jensen & Erik A. Richter
Faculty of Pharmaceutical Sciences, University of British Columbia, Vancouver, BC, Canada
Thomas J. Velenosi
Departments of Integrative Biology and Pharmacology, Houston Medical School, Houston, TX, 77030, USA
Dmitry Akhmedov & Rebecca Berdeaux
Mouse Metabolism Core, National Institute of Diabetes and Digestive and Kidney Diseases, Bethesda, MD, 20892, USA
Oksana Gavrilova
Departments of Genetics and Development, Vagelos College of Physicians and Surgeons, Columbia University, New York, NY, USA
Gerard Karsenty
Metabolic Diseases Branch, National Institute of Diabetes and Digestive and Kidney Diseases, Bethesda, MD, 20892, USA
Min Chen & Lee S. Weinstein
Muscle Physiology and Metabolism Group, German Institute of Human Nutrition, Potsdam-Rehbrücke, Nuthetal, Germany
Maximilian Kleinert

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Jaroslawna Meister
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Derek B. J. Bone
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Jonas R. Knudsen
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Min Chen
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Contributions

J.M., D.B.J.B., and J.W. designed the study. J.M., D.B.J.B., J.R.K., L.F.B., T.J.V., D.A., R.J.L., A.H.C., O.G., and Y.C. carried out experiments and interpreted and analyzed experimental data. R.B., G.K., M.C., and L.S.W. provided mutant mouse models and helpful advice. M.K., T.E.J., and E.A.R. supervised and performed part of the studies and provided critical guidance regarding the preparation of the manuscript. J.M., D.B.J.B., and J.W. wrote the manuscript.

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Correspondence to Jaroslawna Meister or Jürgen Wess.

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Meister, J., Bone, D.B.J., Knudsen, J.R. et al. Clenbuterol exerts antidiabetic activity through metabolic reprogramming of skeletal muscle cells. Nat Commun 13, 22 (2022). https://doi.org/10.1038/s41467-021-27540-w

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Received: 13 January 2021
Accepted: 24 November 2021
Published: 10 January 2022
DOI: https://doi.org/10.1038/s41467-021-27540-w

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