Brown adipose tissue (BAT) dissipates energy through Ucp1-mediated uncoupled respiration and its activation may represent a therapeutic strategy to combat obesity. Here we show that Lkb1 controls BAT expansion and UCP1 expression in mice. We generate adipocyte-specific Lkb1 knockout mice and show that, compared with wild-type littermates, these mice exhibit elevated UCP1 expression in BAT and subcutaneous white adipose tissue, have increased BAT mass and higher energy expenditure. Consequently, KO mice have improved glucose tolerance and insulin sensitivity, and are more resistant to high-fat diet (HFD)-induced obesity. Deletion of Lkb1 results in a cytoplasm to nuclear translocation of CRTC3 in brown adipocytes, where it recruits C/EBPβ to enhance Ucp1 transcription. In parallel, the absence of Lkb1 also suppresses AMPK activity, leading to activation of the mTOR signalling pathway and subsequent BAT expansion. These data suggest that inhibition of Lkb1 or its downstream signalling in adipocytes could be a novel strategy to increase energy expenditure in the context of obesity, diabetes and other metabolic diseases.
The global epidemic of obesity is associated with high risks of metabolic diseases including type 2 diabetes, insulin resistance, heart disease, stroke, hypertension and cancer1. When energy intake consistently exceeds total energy expenditure, the excessive energy is stored in white adipocytes, whose expansion results in obesity. Adipose tissues also play an important role in energy expenditure2. Brown adipose tissue (BAT) is specialized in breaking down lipids to generate heat to defend against hypothermia. This thermogenic property of BAT is mediated by Ucp1, a mitochondria protein that uncouples electron transport from ATP production, leading to generation of heat2,3,4. Recently, a population of Ucp1-expressing thermogenic cells was also identified in WAT. These so-called beige or brite (brown in white) adipocytes can be induced by sympathetic nerve innervation, cold exposure, chemical (or hormonal) stimulations and alterations in gene expression1,5,6,7,8,9,10,11,12,13,14,15,16. Beige adipocytes are similar to classical brown adipocytes in that they can burn lipids to produce heat, but can be distinguished from classical brown adipocytes by the expression of specific cell surface markers (Tmem26 and CD137)2.
The thermogenic activity of brown and beige adipocytes has been reported to increase energy expenditure and thus counteracts obesity5,17,18,19. In contrast, transgenic mice that are genetically ablated of BAT are prone to the development of obesity20. Notably, beige and brown adipocytes have recently been detected in adult humans21,22,23,24,25,26,27. The prevalence of beige or brown adipocytes in adult human is inversely correlated with body mass index, adiposity and fasting plasma glucose level24, indicating these UCP1-expressing adipocytes play an important role in regulating metabolism. Moreover, activation of BAT/beige adipocytes thermogenesis by cold exposure, or by β3-adrenergic receptor agonist activation, has been linked to increased energy expenditure, reduced adiposity and lower plasma lipids21,25,28. Therefore, understanding the molecular regulation of brown and beige adipocyte activity and biogenesis may lead to novel strategies to control energy homoeostasis.
The serine/threonine kinase 11 (Stk11), commonly known as liver kinase b1 (Lkb1), is initially identified as a tumour suppressor mutated in Peutz–Jeghers syndrome29,30. Lkb1 plays important roles in various biological processes including cellular energy metabolism31, cell polarity32 and cancer initiation and progression33. Tissue-specific deletions of Lkb1 in the liver34, pancreas32,35, heart36 and skeletal muscle37,38,39,40 have revealed that Lkb1 functions to control glucose homoeostasis and energy metabolism in various tissues. Recently, Zhang et al.41 generated Fabp4-Cre mediated Lkb1 knockout (KO) mouse model. Interestingly, Fabp4-Cre failed to induce Lkb1 deletion in BAT in that model41, thus the role of Lkb1 in BAT has yet to be determined. In this study, we used a mature adipocyte-restricted adiponectin-Cre (abbreviated as Adipoq-Cre) mouse model42,43 to specifically delete Lkb1 in WAT and BAT. We found that Adipoq-Cre induces efficient deletion of Lkb1 in various adipose tissues including BAT, and results in robust metabolic phenotypes. We further elucidated the molecular mechanisms underlying the role of Lkb1 in BAT. Our results demonstrate that Lkb1 is a critical regulator of BAT growth and function, and suggest that Lkb1 signalling may be therapeutically targeted to counteract obesity, diabetes and other metabolic diseases.
Adipocyte-specific deletion of Lkb1 expands BAT
To directly investigate the role of Lkb1 in adipose tissues, we used the Cre-loxP recombination system involving Adipoq-Cre and Lkb1flox/flox mice (Fig. 1a). Previous studies verified the adipocyte-specific expression pattern of Adipoq-Cre42,43. Thus, in the Adipoq-Cre/ Lkb1flox/flox mice (abbreviated as Adipoq-Lkb1) all adipocytes should be deleted of exons 3–6 of the Lkb1 gene, leading to loss of the kinase domain and premature translational termination of the Lkb1 protein (Fig. 1a). Western blot and quantitative PCR analysis confirmed the efficient and specific deletion of Lkb1 in BAT and WAT (Fig. 1b,c), but not in non-adipose tissues including spleen, lung, kidney, liver, heart and muscle (Supplementary Fig. 1a).
The Adipoq-Lkb1 mice were born at expected Mendelian ratio, and morphologically indistinguishable from their wild-type (WT) littermates. Notably, the BAT size of the female and male Adipoq-Lkb1 mice was substantially enlarged: equivalent to 204 and 177% of the BAT weight in sex-matched WT mice, respectively (Fig. 1d,e). The size and weight of various WAT depots, however, were identical in the WT and Adipoq-Lkb1 mice (Fig. 1d,f). In addition, the weights of other non-adipose tissues were not affected by Adipoq-Lkb1 deletion (Supplementary Fig. 1b,c). When fed on regular chow diet, the Adipoq-Lkb1 mice had similar body weights, growth curves and energy intakes as the WT littermates (Fig. 1g,h). Taken together, deletion of Lkb1 in adipocytes caused a specific expansion of BAT but not WAT.
We next examined whether the increased BAT mass in Adipoq-Lkb1 mice is due to hypertrophy (increase in adipocyte size) or hyperplasia (increase in adipocyte number). Hematoxylin-eosin (H&E) staining revealed an obvious increase in adipocyte size in Adipoq-Lkb1 BAT compared with WT BAT, accompanied by increased abundance of lipid droplets and infiltration of oligolocular and unilocular adipocytes (Fig. 2a). Nuclei densities (nuclei number per unit area) were also significantly lower in the Adipoq-Lkb1 mice compared with the WT mice (Fig. 2a,b), confirming larger adipocyte size in the KO mice. In addition, genomic DNA content per BAT depot was higher in the Adipoq-Lkb1 mice compared with the WT mice (Fig. 2c), suggesting that the Adipoq-Lkb1 BAT contains more cells per depot than the WT BAT depots. To investigate whether increased cell proliferation contributes to the hyperplasia, we used Ki67 staining to mark proliferating cells. At P2 stage when BAT undergoes fast growth, the Adipoq-Lkb1 BAT contains a higher percentage of Ki67+ cells than WT BAT (Supplementary Fig. 2a). This observation suggests that Lkb1 deletion in post-mitotic adipocytes may exert paracrine or contact-dependent effects on progenitor cell proliferation. These data indicated that expansion of BAT mass in the Adipoq-Lkb1 mice is a consequence of combined hypertrophy and hyperplasia of adipocytes.
Lkb1 KO upregulates BAT-specific genes
We further analysed the expression of a panel of adipogenic genes. Despite the apparent infiltration of unilocular white adipocyte-like cells, the Adipoq-Lkb1 BAT expressed higher levels of Ucp1 than the WT BAT (Fig. 2d,e). Consistently, the mRNA levels of BAT-selective Prdm16, Dio2 and Pgc1a genes were significantly higher in the Adipoq-Lkb1 BAT than the WT BAT (Fig. 2d,e). The mRNA levels of the pan-adipocyte genes Pparg and Adipoq were indistinguishable between the two genotypes (Fig. 2d,e). Consistent with the observed infiltration of unilocular adipocytes, the expression of WAT-selective Trim14 gene was also higher in the Adipoq-Lkb1 than WT BAT, but the expression of Agt and Retn, two other WAT-selective genes, was not affected (Fig. 2d,e). These data indicate that the expansion of BAT in Adipoq-Lkb1 mice is associated with higher expression levels of BAT-selective genes.
To investigate whether deletion of Lkb1 affects brown adipocyte differentiation in culture, we isolated SVF cells from BAT depots of WT and Adipoq-Lkb1 mice. Lkb1 deletion marginally promoted brown adipocytes differentiation and triglyceride (TG) accumulation (Supplementary Fig. 3a,b). Consistent with the in vivo data, Lkb1 deficiency markedly increased the expression of Ucp1 and Pgc1a in cultured brown adipocytes (Supplementary Fig. 3c,d). By contrast, overexpression of Lkb1 suppressed brown adipocyte differentiation and TG accumulation (Supplementary Fig. 4a–c), accompanied by apparent inhibition of Prdm16, Pgc1a, Ucp1, Pparg, C/ebpa and Fabp4 expression (Supplementary Fig. 4d). Taken together, these results indicate that deletion of Lkb1 promotes brown adipocyte proliferation, differentiation and gene expression in vivo and in vitro.
Deletion of Lkb1 induces browning of subcutaneous WAT
We next investigated how deletion of Lkb1 affects WAT depots. Although the appearance and mass of inguinal WAT (iWAT), anterior subcutaneous WAT (asWAT) and epididymal WAT (eWAT) were indistinguishable between the Adipoq-Lkb1 and WT mice (Fig. 1), H&E staining revealed that the Adipoq-Lkb1 iWAT contains numerous small multilocular cells resembling beige adipocytes (Supplementary Fig. 5a). However, the genomic DNA contents per iWAT depot were identical in WT and Adipoq-Lkb1 mice (Supplementary Fig. 5b). These results suggest that Lkb1 deletion does not alter the overall number and size of white adipocytes.
Consistent with the appearance of multilocular cells in iWAT, the beige/brown adipocyte-specific Ucp1 protein was expressed at much higher levels in the subcutaneous WAT depots of Adipoq-Lkb1 than those of WT mice (Supplementary Fig. 5c,d). Furthermore, compared with the WT counterparts, Adipoq-Lkb1 iWAT and asWAT expressed higher mRNA levels of BAT signature markers Ucp1 and Pgc1a, but not WAT markers Adipoq and Lep (Supplementary Fig. 5c,d). Interestingly, deletion of Lkb1 did not affect the expression of Ucp1 in eWAT (Supplementary Fig. 5e). These data suggest that lack of Lkb1 robustly induces browning of subcutaneous WAT but not visceral WAT.
Cold stress stimulates beige adipocytes formation and browning of WAT16,25. The rectal temperatures of the Adipoq-Lkb1 mice were higher than those of WT mice after cold exposure for 3 h, even though they had identical rectal temperatures at the room temperature (Supplementary Fig. 5f). In addition, cold exposure elicited a more profound induction of Ucp1 expression in iWAT of Adipoq-Lkb1 mice compared with the WT mice (Supplementary Fig. 5g). The mRNA levels of Ucp1 and Pgc1a were eight- and six-fold higher, respectively, in the iWAT of Adipoq-Lkb1 mice compared with WT mice after cold exposure (Supplementary Fig. 5h). These results indicate that Adipoq-Lkb1 mice are more adaptive to cold-induced browning.
We further analysed SVF cells from iWAT of WT and Adipoq-Lkb1 mice. Deletion of Lkb1 promoted adipogenic differentiation and TG accumulation, as revealed by Oil red O staining (Supplementary Fig. 6a,b). Notably, the protein level of Ucp1 was significantly higher in Lkb1 KO than WT adipocytes (Supplementary Fig. 6c). The mRNA levels of the browning markers Ucp1, Cidea, Pgc1a and Ppara, were increased by 62-, 10-, 4- and 4-fold, respectively, in the Lkb1 KO adipocytes compared with the WT cells (Supplementary Fig. 6d). Conversely, overexpression of Lkb1 inhibited differentiation of WAT SVF cells and TG accumulation (Supplementary Fig. 7a–c), accompanied by apparent inhibition of Ucp1, Pparg, C/ebpa and Fabp4 expression, but not Prdm16 and Pgc1a expression (Supplementary Fig. 7d). These results indicate that the deletion of Lkb1 promotes browning of WAT in a cell autonomous manner.
Improved glucose metabolism in Adipoq-Lkb1 mice
As brown and beige adipocytes improve glucose metabolism and insulin sensitivity19,44, we next examined whether expansion of BAT and browning of WAT in the Adipoq-Lkb1 mice elicits beneficial metabolic effects. We conducted glucose tolerance tests (GTT) and insulin tolerance tests (ITT). Compared with the WT littermates, Adipoq-Lkb1 mice had lower blood glucose levels after intraperitoneal (i.p.) injection of glucose (Fig. 3a). The area under curve of the Lkb1 KO mice was significantly smaller than those of WT mice (Fig. 3b). We also observed faster insulin-stimulated glucose clearance in Adipoq-Lkb1 mice compared with the WT mice (Fig. 3c). In addition, the Adipoq-Lkb1 mice had higher rates of oxygen consumption and carbon dioxide production, and expended more energy compared with the WT mice (Fig. 3d–f; Supplementary Fig. 8a–c). Taken together, these results suggest that adipocyte-specific deletion of Lkb1 improves systemic insulin sensitivity, glucose tolerance and energy metabolism. However, we can’t exclude the possibility that alterations in physical activity may have also partially contributed to the higher energy expenditure, despite similar motor behaviours being observed (Supplementary Movie 1).
Adipoq-Lkb1 mice are resistant to HFD-induced obesity
To examine the long-term effect of Lkb1 deletion on energy metabolism, we fed the mutant mice and WT littermates with high-fat diet (HFD). The Adipoq-Lkb1 mice appeared much leaner than the WT littermates after HFD feeding (Fig. 4a). The body weight of Adipoq-Lkb1 mice, which was similar to WT mice before HFD feeding, was consistently lighter than the WT mice after 3 weeks on HFD (Fig. 4b), even though larger amounts of food were consumed (Fig. 4c). After fed with HFD for 12 weeks, the average body weight of WT was 44.8±1.8 g, while that of the Adipoq-Lkb1 mice was only 33.7±1.0 g (Supplementary Fig. 9a). The body weight difference was mainly due to a reduction of adipose and liver mass in the Adipoq-Lkb1 mice (Fig. 4d; Supplementary Fig. 9b,c). Compared with WT mice, the Adipoq-Lkb1 mice retained better glucose tolerance and higher insulin sensitivity after HFD feeding (Fig. 4e,f). The fasting glucose levels of the Adipoq-Lkb1 mice were also lower than that of WT mice (Supplementary Fig. 9d–h). In addition, the Adipoq-Lkb1 mice retained higher respiration rate and energy expenditure after HFD treatment (Fig. 4g,h). Furthermore, the lipid content was much lower in liver of Adipoq-Lkb1 mice than in WT mice, especially after HFD feeding (Fig. 4i,j; Supplementary Fig. 9i). These results together suggest that BAT expansion and the browning of WAT in Adipoq-Lkb1 mice increases energy expenditure and protects mice from HFD-induced obesity and fatty liver.
To examine whether the systemic metabolic changes were due to enhance energy expenditure of adipocytes, we analysed oxygen consumption rate (OCR) of adipocytes differentiated from Adipoq-Lkb1 and WT SVF cells. The basal respiration, uncoupled respiration after Oligomycin inhibition of ATP synthesis and maximal respiration after stimulation with carbonyl cyanide 4-(trifluoromethoxy)phenylhydrazone (FCCP) were all significantly higher in Adipoq-Lkb1 brown adipocytes than in WT adipocytes (Supplementary Fig. 10a,b). Likewise, Adipoq-Lkb1 iWAT adipocytes exhibited higher basal and uncoupled OCR (Supplementary Fig. 10c,d).
To investigate whether the improved energy expenditure of Adipoq-Lkb1 mice requires Ucp1 function, we analysed mice fed on a HFD and housed at 30 °C (thermoneutrality) to block Ucp1 function. Interestingly, the body weights of Lkb1 KO mice were similar to the WT mice until 7 weeks after HFD feeding (Supplementary Fig. 11a,b). In addition, WT and Adipoq-Lkb1 mice had similar glucose tolerance and insulin sensitivity (Supplementary Fig. 11c,d). Furthermore, thermoneutrality treatment abolished the beneficial metabolic phenotypes of Adipoq-Lkb1 mice observed at room temperature (Supplementary Fig. 11e–g). However, there is a non-significant trend that the Adipoq-Lkb1 mice still maintain a lower body weight, better glucose tolerance and insulin sensitivity (Supplementary Fig. 11b–d). Given this observation, we conclude that the higher energy expenditure in the Lkb1 KO mice is predominantly, but not exclusively, Ucp1 dependent. Other factors such as skin, fur and tail that influencing cold perception may also play a role45, even though we did not detect any morphological abnormality in skin, fur and tail in the Lkb1 KO mice.
Lkb1 KO induces BAT expansion through AMPK-mTOR pathway
To investigate how Lkb1 deficiency leads to the expansion of BAT, we examined the canonical Lkb1-AMPK-mTOR pathway involved in controlling cell growth. Deletion Lkb1 inhibited the kinase activity of AMPK in BAT (Supplementary Fig. 12a) without altering the activity of SIK (Supplementary Fig. 12a), another Lkb1 substrate that has been shown to regulate adipogenesis and insulin signalling46,47. In addition, Lkb1 deletion reduced the levels of phosphorylated AMPK (pAMPK, T172) and increased phosphorylated S6 (pS6, S240/244) in BAT (Supplementary Fig. 12b), suggesting activation of the mTOR pathway.
As mTOR activation promotes adipogenesis and inactivation reduces fat mass48,49, we further examined whether Lkb1 regulate BAT size through the mTOR pathway. To test this, we established the Adipoq-Cre/ Lkb1flox/flox/ mTORflox/flox mice (adipocyte-specific Lkb1 and mTOR double KO mice, abbreviated as DKO). The body weights of WT, Adipoq-Lkb1 and DKO were similar (Supplementary Fig. 12c) but the BAT expansion phenotype in Adipoq-Lkb1 is rescued by DKO (Supplementary Fig. 12d–f). Furthermore, DKO rescued or reversed the expression pattern of adipogenic and BAT-selective genes in Adipoq-Lkb1 BAT (Supplementary Fig. 12g). These results suggest that deletion of Lkb1 promotes BAT expansion through dampening AMPK activity and activating the mTOR pathway.
Lkb1 deletion induces nuclear translocation of CRTC3
To understand the molecular mechanism through which Lkb1 regulates Ucp1 gene expression, we examined the CRTC3 signalling pathway, which is highly expressed in adipocytes and has important functions in fine-tuning glucose and lipid metabolism, and mitochondrial biogenesis50,51,52. Strikingly, Lkb1 deletion led to apparent nuclear translocation of CRTC3 (Fig. 5a,b), without affecting its total protein levels in adipocytes or adipose tissues (Supplementary Fig. 13a–d). Immunostaining revealed intense CRTC3 signals in the nucleus of Lkb1 KO adipocytes, but not WT adipocytes (Fig. 5a). These results suggest that the higher Ucp1 expression in the Adipoq-Lkb1 KO mice is correlated to CRTC3 nuclear localization.
To understand how Lkb1 affects the intracellular compartmentalization of CRTC3, we used co-immunoprecipitation (Co-IP) to examine whether these two proteins interact. Indeed, we detected robust pull-down of CRTC3 by Lkb1 antibody in 293T cells after overexpression of these genes and vice versa (Fig. 5c–e). Furthermore, we detected endogenous interaction between CRTC3 and Lkb1 proteins in differentiated BAT SVF cells, 3T3-L1 cells and adipose tissues (Supplementary Fig. 14). These data suggest that Lkb1 interacts with CRTC3, and subsequently regulates its intracellular localization.
CRTC3 binds C/EBPβ to increase its transcriptional activity
We further investigated how nuclear translocation of CRTC3 regulates Ucp1 gene expression. CRTC3 has been shown to bind to the basic leucine zipper (bZIP) domain of CREB to enhance its transcriptional activity53,54. As C/EBPβ is also a member of the bZIP transcription factor family55 and is essential for brown adipocytes differentiation and Ucp1 expression56, we asked whether CRTC3 binds C/EBPβ to regulate BAT gene expression. We first confirmed that overexpression of C/EBPβ in brown adipocytes significantly increased the expression of brown fat related genes including Ucp1, Prdm16 and Pgc1a (Supplementary Fig. 15a). In addition, chromatin immunoprecipitation (ChIP) and luciferase reporter assay indicated that C/EBPβ directly binds to the promoter of Ucp1 to enhance Ucp1 gene transcription (Supplementary Fig. 15b,c).
We then performed Co-IP experiments after overexpression in 293T cells and found that C/EBPβ can be pulled down by CRTC3 and vice versa (Fig. 6a–c). Likewise, endogenous interactions between CRTC3 and C/EBPβ were also found in differentiated BAT SVF cells, 3T3-L1 and BAT (Supplementary Fig. 16), suggesting that CRTC3 physically interacts with C/EBPβ. To examine the function of this interaction, we transfected 293T cells with pcNDA-Flag-CRTC3, pcDNA-C/EBPβ and PGL3–Ucp1 (Ucp1 luciferase reporter) plasmids in a combinatorial fashion. Importantly, co-transfection of CRTC3 markedly increased the transcriptional activity of C/EBPβ on the Ucp1 promoter (Fig. 6d), indicating CRTC3 binds to C/EBPβ and regulates C/EBPβ transcriptional activity.
To directly interrogate whether CRTC3 is necessary to mediate the effects of Lkb1 deletion on Ucp1 expression, we knocked-down CRTC3 in BAT SVF isolated from Lkb1flox/flox mice. Remarkably, we found that knockdown CRTC3 abolished the induction of Ucp1 expression by Lkb1 deletion in the subsequently differentiated brown adipocytes (Fig. 6e). Therefore, we conclude that Lkb1 deletion promotes CRTC3 nuclear translocation, where CRTC3 interacts with C/EBPβ to upregulate Ucp1 expression (Fig. 6f).
In this study, we discovered that adipocyte-specific deletion of Lkb1 leads to the expansion of classical BAT and increases the expression of Ucp1 in BAT and sWAT. This subsequently improves glucose metabolism, increases energy expenditure and protects mice from HFD-induced obesity. We delineated that Lkb1 affects the BAT expansion through AMPK-mTOR pathway and provided biochemical evidence that Lkb1 interacts with CRTC3 and deletion of Lkb1 promotes CRTC3 nuclear translocation. Finally, we showed that nuclear CRTC3 binds to C/EBPβ and promotes its transcriptional activity, and Lkb1 deletion upregulates Ucp1 level through CRTC3. It is worth mentioning that although the data reported in some figures (for example, Fig. 2) are derived from male mice, the Adipoq-Lkb1 KO females exhibit identical phenotype. These results from both genders reveal a critical role of Lkb1 signalling pathway in regulating BAT development and whole-body insulin sensitivity and energy metabolism.
We used a highly adipocyte-specific Adipoq-Cre mouse model42,43 to drive the deletion of Lkb1. Our results are in contrast to the phenotypes observed in Fabp4-Cre-driven Lkb1 KO mice (termed Fabp4-Lkb1 KO henceforth), which develop lipodystrophy in WAT and die prematurely41. As Fabp4-Cre is expressed in mature adipocytes as well as preadipocytes (adipo-progenitors), the lipodystrophy of WAT in the Fabp4-Lkb1 KO mice may be due to the key role of Lkb1 in white preadipocyte survival and differentiation. In addition, the leaky expression of Fabp4-Cre in non-adipose tissues including endothelial cells42,57 may have led to off-target effects that contributed to the premature death of the Fabp4-Lkb1 KO mice. Indeed, it was reported that endothelium-specific deletion of Lkb1 in mice results in premature death58,59. As white adipocyte differentiation and growth predominantly occur at postnatal stages, the premature death of the Fabp4-Lkb1 KO mice may have prevented the normal growth of WAT independent of Lkb1 function in adipose per se. Surprisingly, Fabp4-Cre fails to induce Lkb1 deletion in BAT, even though lineage tracing experiments clearly demonstrate that Fabp4-Cre marks a population of progenitors and all mature adipocytes in the BAT60. Compared with the Fabp4-Lkb1 KO, our mouse model not only bypasses the premature lethality but also results in robust deletion of Lkb1 in both WAT and BAT, thus provides an excellent opportunity to unbiasedly assess the role of Lkb1 in adipocytes.
In our indirect calorimetry study, O2 consumption and CO2 production were normalized by body weight (BW). Other normalization standards in the field include lean mass and per animal61. Given that the KO and WT mice have similar BW when fed on chow diet, using BW or per animal for normalization should give the same result. However, the KO mice were lighter than the WT mice after HFD feeding, mainly due to changes in fat and liver mass, we choose to normalize the values to BW to reflect such changes. Recently, Tschoep et al.61 suggested that combining effects of different tissues and using analysis of covariance would facilitate unbiased comparison of energy expenditure measurements across studies.
It is interesting that Adipoq-Lkb1 KO BAT on one hand appears to be morphologically whitened but on the other hand expresses higher levels of Ucp1 and exhibits higher thermogenic activities (based on OCR analysis). This paradoxical observation suggests that thermogenic activity of adipocytes is not always associated with the size and number of lipid droplets. In the Lkb1 KO mice, hypertrophy of brown adipocytes may have simultaneously increased their lipid storage (size of lipid droplets) and thermogenic capacities. Supporting this idea, both white and brown adipocytes are hypertrophic (that is, contain larger lipid droplets) in the Adipoq-Pten KO mice but the mice have enhanced insulin sensitivity62. Alternatively, the increased lipid storage in Adipoq-Lkb1 KO brown adipocytes may be an adaptive mechanism to allow sufficient lipid supply to match a greater rate of lipid utilization. It is well-known that lipolysis of triacylglycerol (lipid droplets) generates free fatty acids that subsequently activates Ucp1 (ref. 63). Other groups have reported that browning conditions (such as β3-adrenergic receptor activation and cold exposure) elevate fatty acid synthase (FAS) in BAT to promote free fatty acids re-esterification and triacylglycerol formation64,65. Thus, concomitant increases in lipid storage and utilization may explain the BAT phenotypes in the Adipoq-Lkb1 KO mice.
Loss function of Lkb1 in WAT and BAT cells promoted adipocyte differentiation and lipid accumulation, accompanied by increased expression of brown/beige specific genes. Conversely, Lkb1 overexpression reduced the lipid accumulation, and suppressed expression of brown/beige-specific genes. However, we noted that the extent of changes in differentiation markers was lesser than the extent of changes in BAT-specific gene expression. Therefore, changes in BAT marker gene expression may be partially due to alterations in overall differentiation.
AMPK is a canonical substrate of Lkb1 and an energy sensor through interaction with mTOR signalling pathway66. We found that deletion of Lkb1 decreases the activity and phosphorylation of AMPK while increasing the phosphorylation of S6, an established downstream target of mTOR. This result suggests that Lkb1 regulates mTOR pathway through AMPK in adipocytes. As mTOR pathway plays positive roles in regulating the fat mass and fat cell size48,49,67, augmentation of mTOR signalling in the Adipoq-Lkb1 KO mice explains the BAT expansion phenotype. Double deletion of Lkb1 and mTOR provides the definitive proof that Lkb1 regulates BAT mass through mTOR.
We discovered a novel interaction between Lkb1 and CRTC3 that controls the intracellular localization of CRTC3, a transcriptional co-activator that is highly expressed in adipose tissues51. The CRTC family proteins possess a highly conserved N-terminal CREB-binding domain, which interacts with the bZIP domain of CREB and to regulate its activity53,68,69,70. Under basal conditions, CRTC1 and CRTC2 are mainly sequestered in the cytoplasm through phosphorylation and interactions with 14-3-3 proteins51,54, while CRTC3 is thought to be mainly localized in the nucleus70. However, we found that CRTC3 was mainly localized in cytoplasm of brown adipocytes in the WT mice, and Lkb1 deletion induced nuclear translocation of CRTC3. Dephosphorylation-mediated nuclear translocation of CRTCs is a critical and conserved step governing their function in upregulating CREB target genes53,54. Previous studies have shown that Lkb1 substrates such as AMPK and SIK can phosphorylate CRTCs and inhibit CREB-mediated gene expression70,71,72. As such, CRTC2 is a critical downstream target of LKB1/AMPK signals in the regulation of liver gluconeogenesis34. Here we found that Lkb1 directly interacts with CRTC3. We speculate that the protein kinase domain of Lkb1 interacts with the central regulatory region of CRTC3, where Lkb1 phosphorylates the Ser residue of CRTC3 to regulate its translocation between cytoplasm and nuclear. On the basis of a previous study73 and online protein software (Uniport) analysis, phosphorylation of Ser62, Ser162, Ser329, Ser370, Ser391 and Ser443 may be involved in the intracellular localization of CRTC3. However, pinpointing the exact Lkb1 phosphorylation site requires further biochemical analysis.
We demonstrate in this study that CRTC3 interacts with C/EBPβ to promote its transcriptional activity. C/EBPβ has been reported to play an important role in regulating BAT differentiation and gene expression56. Consistently, we found that overexpression C/EBPβ in BAT cells potently induces expression of BAT-related genes. ChIP and luciferase assays further showed that C/EBPβ directly binds to Ucp1 promoter to upregulate its expression. Importantly, luciferase assay indicates that CRTC3 upregulates the transcriptional activity of C/EBPβ on the Ucp1 promoter, thus demonstrating the functional significance of the CRTC3-C/EBPβ interaction.
Our conclusion that Lkb1 KO upregulates Ucp1 expression through CRTC3 is supported by knockdown assays in which knocking down CRTC3 in Lkb1 null adipocytes abolishes Ucp1 upregulation. Likewise, in muscle and liver cells, CRTC3 markedly induce PGC-1 (an upstream regulator of Ucp1) transcription and mitochondrial biogenesis74,75. Interestingly, previous reports have shown that whole-body KO of CRTC3 increases energy expenditure and protect the mutant mice from obesity and hepatic steatosis51, which appear to contradict our observation that CTRC3 knockdown prevents Ucp1 upregulation in Lkb1 KO adipocytes. However, the previous study is inconsistent to the overall phenotype of the Adipoq-Lkb1 KO mice in which the total protein levels of CRTC3 were not affected. Instead, what seems to be most important in adipocytes is the translocation of CRTC3 into the nucleus, where it acts as a novel co-activator of C/EBPβ to regulate Ucp1 gene expression.
All procedures involving mice were approved by Purdue University Animal Care and Use Committee. The Adipoq-Cre (stock #010803), Lkb1flox/flox (stock #014143) and mTORflox/flox (stock #011009) mice were purchased from Jackson Laboratory (Bar Harbor, ME). Mice were in a C57BL/6J background and housed in the animal facility with free access to water and standard rodent chow food or HFD (TD.06414 Harlan). PCR genotyping was done using protocols described by the supplier. Food intake assay was calculated by measuring food consumption weekly. Unless otherwise indicated, 2–5 months old adult mice of both sexes were analysed in this study.
Indirect calorimetry study
Oxygen consumption (VO2), carbon dioxide production (VCO2), respiratory exchange ratios and heat production were measured by using indirect calorimetry system (Oxymax, Columbus Instruments), installed under a constant environmental temperature (22 or 30 °C) and a 12-h light (06:00–18:00 hours), 12-h dark cycle (18:00–06:00 hours). Mice in each chamber had free access to food and water. The raw data were normalized by body weight and the histograms of day (06:00–18:00 hours) and night (18:00–06:00 hours) values were the mean value of all points measured during the 12-h period.
Blood glucose measurements
For GTT, mice were given i.p. injection of 100 mg ml−1 D-glucose (2 g kg−1 body weight) after overnight fasting, and tail blood glucose concentrations were measured by a glucometer (Accu-Check Active, Roche). For ITT, mice were fasted for 4 h before i.p. administration of human insulin (Santa Cruz) (0.75 U per kg body weight), and tail blood glucose concentrations were monitored. For both GTT and ITT, each mouse was singly caged with blinded cage number and random orders.
H&E staining and immunostaining
Adipose tissues from the WT and Adipoq-Lkb1 mice were fixed in 10% formalin for 24 h at room temperature. Then the tissues were embedded into paraffin, blocked and cut at 3–10 μm for H&E staining and immunostaining. For H&E staining, the sections were deparaffinized, rehydrated and the nuclei stained with haematoxylin for 15 min. Sections were then rinsed in running tap water and stained with eosin for 1 min, dehydrated and mounted. Whole-slide digital images were collected at × 20 magnification with an Aperio Scan Scope slide scanner (Aperio, Vista, CA). Scanned images of H&E staining were analysed by Photoshop CS3 to calculate nuclei numbers. For immunostaining, the sections were blocked with blocking buffer containing 5% goat serum, 2% BSA, 0.2% triton X-100 and 0.1% sodium azide in PBS for 1 h after deparaffinized and antigen retrieval. Then the samples were incubated with CRTC3 (Cell Signalling, C35G4) and Ki67 (Abcam, ab-16667) primary antibodies diluted in blocking buffer overnight. After washing with PBS, the samples were incubated with secondary antibodies and DAPI for 45 min at room temperature. Fluorescent images were captured as single-channel grayscale images using a Leica DM 6000B fluorescent microscope with a × 20 objective (NA 0.70). Images for WT and conditional KO samples were captured using identical parameters and both WT and mutant images were adjusted identically in Photoshop.
Primary BAT and WAT SVF cells were isolated using collagenase digestion and followed by density separation. Briefly, the interscapular brown adipose and inguinal white adipose were minced and digested in 1.5 mg ml−1 collagenase at 37 °C for 0.5 and 1 h, respectively. The digestions were terminated with DMEM containing 10% FBS, and filtered through 100-μm filters to remove connective tissues and undigested trunks of tissues. Cells were then centrifuged at 450g for 5 min to separate the SVF cells in the sediment and lipid-containing adipocytes in the floating layer. The freshly isolated SVF cells were seeded and cultured in growth medium containing DMEM, 20% FBS, 1% penicillin/streptomycin (P/S) at 37 °C with 5% CO2 for 3 days, followed by feeding with fresh medium every 2 days. The BAT cell line (kindly provided by Professor Yongxu Wang, University of Massachusetts Medical School), were cultured in same condition as SVF cells, while 3T3-L1 (ATCC) and HEK293T (ATCC) were cultured in DMEM with 10% FBS. For SVF cell and BAT cell line adipogenic differentiation, the cells were induced with induction medium contains DMEM, 10% FBS, 2.85 μM insulin, 0.3 μM dexamethasone, 1 μM rosiglitazone, and 0.63 mM 3-isobutyl-methylxanthine for 3 days on confluence and then differentiated in differentiation medium contains DMEM, 10% FBS, 200 nM insulin and 10 nM T3 for 4 days until adipocytes mature. To avoid the effect of cell density on adipogenic differentiation, cells were induced to differentiate when they reach 90% confluence. For 3T3-L1 adipogenic differentiation, cells of 100% confluence were kept in growth medium for 2 days then induced with induction medium for 2 days, after that differentiated in differentiation medium (without T3) for 6 days. Mycoplasma was certified by ATCC when cells were purchased. All cell lines were periodically tested for identity using PCR and by morphological features.
Oil red O staining
Cultured cells were washed with PBS and fixed with 10% formaldehyde for 15 min at room temperature. Then the cells were stained using the Oil red O working solutions containing 6 ml Oil red O stock solution (5 g l−1 in isopropanol) and 4 ml ddH2O for 30 min. After staining, the cells were washed with 60% isopropanol and pictured. Triglycerides were extracted from Oil Red O-stained adipocytes with 100% isopropanol, and the triglyceride contents were analysed by measuring the optical density at 490 nm (OD 490).
Total RNA extraction and real-time PCR
Total RNA was extracted from cells or tissues using Trizol Reagent according to the manufacturer’s instructions. RNA was treated with RNase-free DNase l to remove contaminating genomic DNA. The purity and concentration of total RNA were measured by a spectrophotometer (Nanodrop 3000, Thermo Fisher) at 260 and 280 nm. Ratios of absorption (260/280 nm) of all samples were between 1.8 and 2.0. Then 5 μg of total RNA were reversed transcribed using random primers and MMLV reverse transcriptase. Real-time PCR was carried out with a Roche Lightcycler 480 PCR System using SYBR Green Master Mix and gene-specific primers. Primer sequences are listed in Supplementary Table 1. The 2−ΔΔCT method was used to analyse the relative changes in gene expression normalized against 18S ribosomal RNA as internal control.
Protein extraction and western blot analysis
Total protein was isolated from cells or tissues using RIPA buffer contains 50 mM Tris-HCl (pH 8.0), 150 mM NaCl, 1% NP-40, 0.5% sodium Deoxycholate and 0.1% SDS. The cytoplasm fractions were extract with buffer A contains 10 mM HEPES (pH 7.4), 1 mM KCl, 1 mM EDTA, 1Mm EGTA, 1 mM dithiothreitol, 0.5% Nonidet P-40 and protease inhibitor. After extracted the cytoplasm proteins, the nuclei pellet was washed with buffer A (without Nonidet P-40) and resolved by RIPA buffer for nuclear proteins. Protein concentrations were determined using Pierce BCA Protein Assay Reagent (Pierce Biotechnology). Proteins were separated by SDS–PAGE, transferred to a polyvinylidene fluoride membrane (Millipore Corporation), blocking in 5% fat-free milk for 1 h at RT, then incubated with first antibodies in 5% milk overnight at 4 °C. The CRTC3 antibody was from Cell Signalling (C35G4, 1:1,000), Ucp1 was from Abcam (ab23841, 1:2,000), all other antibodies were from Santa Cruz Biotechnology (Santa Cruz), including Lkb1 (sc-32245, 1:1,000), phosphor-AMPK (sc-33524, 1:1,000), AMPK (sc-25792, 1: 1,000), C/EBPβ (sc-150, 1:1,000), SIK (sc-83754, 1:1,000) and GAPDH (sc-32233, 1:1,000). The horseradish peroxidase (HRP)-conjugated secondary antibody (anti-rabbit IgG, 111-035-003 or anti-mouse IgG; 115-035-003, Jackson ImmunoResearch) or infrared secondary antibody (Alexa Fluor 790 goat anti-mouse IgG, A11357Life Technologies, USA) were diluted 1:5,000 and 1:10,000, respectively. Immunodetection was performed using enhanced chemiluminescence western blotting substrate (Pierce Biotechnology) and detected with FluorChem R System (ProteinSimple). Results shown in the figures are representative results from at least three independent experiments. Uncropped original gel images are available in Supplementary Fig. 17.
Brown fat from the mutant mice were dissected, washed with PBS, minced and fixed with 1% formaldehyde in DMEM for 10 min at room temperature followed by the addition of 125 mM glycine for 5 min at room temperature, after which samples were washed twice with cold PBS and placed in SDS lysis buffer containing 20 mM Tris, 0.1% SDS, 1% Triton-100, 150 mM NaCl, 1 Mm EDTA and protease inhibitor. The samples were further sonicated and diluted for IP with the indicated antibodies (anti-C/EBPβ, 1:50) and incubation at 4 °C overnight. Then, the immunoprecipitates were eluted and reverse crosslinked overnight at 65 °C. DNA fragments were purified using the Cycle Pure kit (Omega Bio-Tek), and quantitative PCR was performed.
HEK293T cells were seeded into 48-well plates 1 day before Lipofectamine 2000–mediated transfection. The pGL3–Ucp1 promoter luciferase plasmid was generated. For transfection of each well, 80 ng Renilla plasmid, 250 ng pGL3–Ucp1 and 500 ng pcDNA-C/EBPβ plasmid (or its blank control plasmid) and/or 500 ng pcDNA-flag-CRTC3 (or its blank control plasmid) were co-transfected following the manufacturer’s instructions. Cells were harvested 36 h after transfection and analysed with the Dual-Luciferase Reporter Assay System (Promega).
Total protein was extracted from HEK293T cells, transfected with pcDNA-flag-CRTC3 or/and pcDNA-C/EBPβ plasmid after 36 h, differentiated 3T3-L1, BAT cell line and BAT. The lysate was precleared with protein A/G agarose at 4 °C for 1 h. Then 2 μg of primary antibody anti-CRTC3, anti-Lkb1, anti-CEBPβ or anti-Flag was added into lysate contains 500 μg total protein and rotating at 4 °C overnight. The next morning added the protein A/G agarose and rotating for 2 h. The samples were washed with cold PBS for three times and collected for western blot.
Adipocyte OCR measurement
Primary SVF cells from BAT and inguinal WAT were isolated and cultured for 3 days before being plated in XF cell culture microplates (Seahorse Bioscience). SVF cells (10,000 cells) were seeded in each well, and each treatment included cells from seven BAT or three WAT replicates. After differentiated 6 d, cultured adipocytes were washed twice and pre-incubated in XF medium (supplemented with 25 mM glucose, 2 mM glutamine and 1 mM pyruvate) for 1–2 h at 37 °C without CO2. The OCR was measured using the XF Extracellular Flux Analyser (Seahorse Biosciences). Oligomycin (2 mM), FCCP (2 mM), and Antimycin A and Rotenone (0.5 μM) were preloaded into cartridges and injected into XF wells in succession. OCR was calculated as a function of time (picomoles per minute).
In vitro kinase assay
IP purified AMPK and SIK from BAT lysates (each sample with the same amount of total protein) was, respectively, incubated with AMARA substrate peptide (Abcam, ab204852), bound on phosphocellulose paper in kinase reaction buffer (50 mM Tris, pH 7.5, 10 mM MgCl2, 2 mM EGTA, 0.5 mM Na3VO4, 100 mM 4-nitrophenyl phosphate di(tris) salt (PNPP), 25 mM dithiothreitol (DTT), 125 μM ATP) supplemented with 10 μCi of [32P] ATP at 30 °C for 30 min. Then the paper was washed, dried and detected by autoradiography.
Trial experiments or experiments done previously were used to determine sample size with adequate statistical power. Measurement values that were beyond the boundary determined by the interquartile range were considered as outliers and were excluded from statistical analyses. Specifically, all data from one WT control mouse were excluded from data analysis in Supplementary Fig. 11 due to blood glucose level at one time point was above the detection range of the glucometer used. No other data were excluded and data are presented as means±s.e.m. Comparisons were made by two-tailed Student’s t-tests. Effects were considered significant at P<0.05. The researchers involved in the study were not completely blinded during sample collection or data analysis.
The data that support the findings of this study are available from the corresponding author on request.
How to cite this article: Shan, T. et al. Lkb1 controls brown adipose tissue growth and thermogenesis by regulating the intracellular localization of CRTC3. Nat. Commun. 7:12205 doi: 10.1038/ncomms12205 (2016).
Cohen, P. et al. Ablation of PRDM16 and beige adipose causes metabolic dysfunction and a subcutaneous to visceral fat switch. Cell 156, 304–316 (2014).
Wu, J., Cohen, P. & Spiegelman, B. M. Adaptive thermogenesis in adipocytes: is beige the new brown? Genes Dev. 27, 234–250 (2013).
Nedergaard, J. & Cannon, B. The changed metabolic world with human brown adipose tissue: therapeutic visions. Cell Metab. 11, 268–272 (2010).
Rosen, E. D. & Spiegelman, B. M. Adipocytes as regulators of energy balance and glucose homeostasis. Nature 444, 847–853 (2006).
Bi, P. et al. Inhibition of Notch signalling promotes browning of white adipose tissue and ameliorates obesity. Nat. Med. 20, 911–918 (2014).
Bostrom, P. et al. A PGC1-alpha-dependent myokine that drives brown-fat-like development of white fat and thermogenesis. Nature 481, 463–468 (2012).
Cao, L. et al. White to brown fat phenotypic switch induced by genetic and environmental activation of a hypothalamic-adipocyte axis. Cell Metab. 14, 324–338 (2011).
Ohno, H., Shinoda, K., Spiegelman, B. M. & Kajimura, S. PPARgamma agonists induce a white-to-brown fat conversion through stabilization of PRDM16 protein. Cell Metab. 15, 395–404 (2012).
Kusminski, C. M., Park, J. & Scherer, P. E. MitoNEET-mediated effects on browning of white adipose tissue. Nat. Commun. 5, 3962 (2014).
Geurts, L. et al. Adipose tissue NAPE-PLD controls fat mass development by altering the browning process and gut microbiota. Nat. Commun. 6, 6495 (2015).
Rosenwald, M., Perdikari, A., Rulicke, T. & Wolfrum, C. Bi-directional interconversion of brite and white adipocytes. Nat. Cell Biol. 15, 659–667 (2013).
Lee, Y. K. & Cowan, C. A. White to brite adipocyte transition and back again. Nat. Cell Biol. 15, 568–569 (2013).
Wang, J. et al. Ablation of LGR4 promotes energy expenditure by driving white-to-brown fat switch. Nat. Cell Biol. 15, 1455–1463 (2013).
Moisan, A. et al. White-to-brown metabolic conversion of human adipocytes by JAK inhibition. Nat. Cell Biol. 17, 57–67 (2015).
Seale, P. et al. Prdm16 determines the thermogenic program of subcutaneous white adipose tissue in mice. J. Clin. Invest. 121, 96–105 (2011).
Dempersmier, J. et al. Cold-inducible Zfp516 activates UCP1 transcription to promote browning of white fat and development of brown fat. Mol. Cell 57, 235–246 (2015).
Crane, J. D. et al. Inhibiting peripheral serotonin synthesis reduces obesity and metabolic dysfunction by promoting brown adipose tissue thermogenesis. Nat. Med. 21, 166–172 (2015).
Rosen, E. D. & Spiegelman, B. M. What we talk about when we talk about fat. Cell 156, 20–44 (2014).
Stanford, K. I. et al. Brown adipose tissue regulates glucose homeostasis and insulin sensitivity. J. Clin. Invest. 123, 215–223 (2013).
Lowell, B. B. et al. Development of obesity in transgenic mice after genetic ablation of brown adipose-tissue. Nature 366, 740–742 (1993).
Cypess, A. M. et al. Activation of human brown adipose tissue by a beta 3-adrenergic receptor agonist. Cell Metab. 21, 33–38 (2015).
Shinoda, K. et al. Genetic and functional characterization of clonally derived adult human brown adipocytes. Nat. Med. 21, 389–394 (2015).
Jespersen, N. Z. et al. A classical brown adipose tissue mRNA signature partly overlaps with brite in the supraclavicular region of adult humans. Cell Metab. 17, 798–805 (2013).
Cypess, A. M. et al. Identification and importance of brown adipose tissue in adult humans. N. Engl. J. Med. 360, 1509–1517 (2009).
van Marken Lichtenbelt, W. D. et al. Cold-activated brown adipose tissue in healthy men. N. Engl. J. Med. 360, 1500–1508 (2009).
Virtanen, K. A. et al. Functional brown adipose tissue in healthy adults. N. Engl. J. Med. 360, 1518–1525 (2009).
Lidell, M. E. et al. Evidence for two types of brown adipose tissue in humans. Nat. Med. 19, 631–634 (2013).
Yoneshiro, T. et al. Recruited brown adipose tissue as an antiobesity agent in humans. J. Clin. Invest. 123, 3404–3408 (2013).
Hemminki, A. et al. A serine/threonine kinase gene defective in Peutz-Jegheus syndrome. Nature 391, 184–187 (1998).
Jenne, D. E. et al. Peutz-Jeghers syndrome is caused by mutations in a novel serine threonine kinase. Nat. Genet. 18, 38–44 (1998).
Nakada, D., Saunders, T. L. & Morrison, S. J. Lkb1 regulates cell cycle and energy metabolism in haematopoietic stem cells. Nature 468, 701–704 (2010).
Granot, Z. et al. LKB1 Regulates Pancreatic beta Cell Size, Polarity, and Function. Cell Metab. 10, 296–308 (2009).
Ji, H. et al. LKB1 modulates lung cancer differentiation and metastasis. Nature 448, 807–810 (2007).
Shaw, R. J. et al. The kinase LKB1 mediates glucose homeostasis in liver and therapeutic effects of metformin. Science 310, 1642–1646 (2005).
Fu, A. et al. Loss of Lkb1 in adult beta cells increases beta cell mass and enhances glucose tolerance in mice. Cell Metab. 10, 285–295 (2009).
Ikeda, Y. et al. Cardiac-specific deletion of LKB1 leads to hypertrophy and dysfunction. J. Biol. Chem. 284, 35839–35849 (2009).
Jeppesen, J. et al. LKB1 regulates lipid oxidation during exercise independently of AMPK. Diabetes 62, 1490–1499 (2013).
Koh, H. J. et al. Skeletal muscle-selective knockout of LKB1 increases insulin sensitivity, improves, glucose homeostasis, and decreases TRB3. Mol. Cell. Biol. 26, 8217–8227 (2006).
Sakamoto, K. et al. Deficiency of LKB1 in skeletal muscle prevents AMPK activation and glucose uptake during contraction. EMBO J. 24, 1810–1820 (2005).
Shan, T. et al. Lkb1 is indispensable for skeletal muscle development, regeneration, and satellite cell homeostasis. Stem Cells 32, 2893–2907 (2014).
Zhang, W., Wang, Q., Song, P. & Zou, M. H. Liver kinase b1 is required for white adipose tissue growth and differentiation. Diabetes 62, 2347–2358 (2013).
Lee, K. Y. et al. Lessons on conditional gene targeting in mouse adipose tissue. Diabetes 62, 864–874 (2013).
Eguchi, J. et al. Transcriptional control of adipose lipid handling by IRF4. Cell Metab. 13, 249–259 (2011).
Orava, J. et al. Different metabolic responses of human brown adipose tissue to activation by cold and insulin. Cell Metab. 14, 272–279 (2011).
Nedergaard, J. & Cannon, B. The Browning of White Adipose Tissue: Some Burning Issues. Cell Metab. 20, 396–407 (2014).
Katoh, Y. et al. Salt-inducible kinase (SIK) isoforms: their involvement in steroidogenesis and adipogenesis. Mol. Cell. Endocrinol. 217, 109–112 (2004).
Okamoto, M., Takemori, H. & Katoh, Y. Salt-inducible kinase in steroidogenesis and adipogenesis. Trends Endocrinol. Metab. 15, 21–26 (2004).
Polak, P. et al. Adipose-specific knockout of raptor results in lean mice with enhanced mitochondrial respiration. Cell Metab. 8, 399–410 (2008).
Um, S. H. et al. Absence of S6K1 protects against age- and diet-induced obesity while enhancing insulin sensitivity. Nature 431, 200–205 (2004).
Qi, L. et al. Adipocyte CREB promotes insulin resistance in obesity. Cell Metab. 9, 277–286 (2009).
Song, Y. et al. CRTC3 links catecholamine signalling to energy balance. Nature 468, 933–U329 (2010).
Wang, Y. G., Vera, L., Fischer, W. H. & Montminy, M. The CREB coactivator CRTC2 links hepatic ER stress and fasting gluconeogenesis. Nature 460, 534–537 (2009).
Bittinger, M. A. et al. Activation of cAMP response element-mediated gene expression by regulated nuclear transport of TORC proteins. Curr. Biol. 14, 2156–2161 (2004).
Altarejos, J. Y. & Montminy, M. CREB and the CRTC co-activators: sensors for hormonal and metabolic signals. Nat. Rev. Mol. Cell. Biol. 12, 141–151 (2011).
Hu, H. M. et al. The C/EBP bZIP domain can mediate lipopolysaccharide induction of the proinflammatory cytokines interleukin-6 and monocyte chemoattractant protein-1. J. Biol. Chem. 275, 16373–16381 (2000).
Tanaka, T., Yoshida, N., Kishimoto, T. & Akira, S. Defective adipocyte differentiation in mice lacking the C/EBPbeta and/or C/EBPdelta gene. EMBO J. 16, 7432–7443 (1997).
Urs, S., Harrington, A., Liaw, L. & Small, D. Selective expression of an aP2/fatty acid binding protein4-Cre transgene in non-adipogenic tissues during embryonic development. Transgenic. Res. 15, 647–653 (2006).
Londesborough, A. et al. LKB1 in endothelial cells is required for angiogenesis and TGF beta-mediated vascular smooth muscle cell recruitment. Development 135, 2331–2338 (2008).
Zhang, W. C. et al. Endothelial cell-specific liver kinase B1 deletion causes endothelial dysfunction and hypertension in mice in vivo. Circulation 129, 1428–1439 (2014).
Shan, T., Liu, W. & Kuang, S. Fatty acid binding protein 4 expression marks a population of adipocyte progenitors in white and brown adipose tissues. FASEB J. 27, 277–287 (2013).
Tschop, M. H. et al. A guide to analysis of mouse energy metabolism. Nat. Methods 9, 57–63 (2012).
Morley, T. S., Xia, J. Y. & Scherer, P. E. Selective enhancement of insulin sensitivity in the mature adipocyte is sufficient for systemic metabolic improvements. Nat. Commun. 6, 7906 (2015).
Nicholls, D. G. & Rial, E. A history of the first uncoupling protein, UCP1. J. Bioenerg. Biomembr. 31, 399–406 (1999).
Mottillo, E. P. et al. Coupling of lipolysis and de novo lipogenesis in brown, beige, and white adipose tissues during chronic beta3-adrenergic receptor activation. J. Lipid Res. 55, 2276–2286 (2014).
Yu, X. X., Lewin, D. A., Forrest, W. & Adams, S. H. Cold elicits the simultaneous induction of fatty acid synthesis and beta-oxidation in murine brown adipose tissue: prediction from differential gene expression and confirmation in vivo. FASEB J. 16, 155–168 (2002).
Lizcano, J. M. et al. LKB1 is a master kinase that activates 13 kinases of the AMPK subfamily, including MARK/PAR-1. EMBO J. 23, 833–843 (2004).
Murakami, M. et al. mTOR is essential for growth and proliferation in early mouse embryos and embryonic stem cells. Mol. Cell. Biol. 24, 6710–6718 (2004).
Iourgenko, V. et al. Identification of a family of cAMP response element-binding protein coactivators by genome-scale functional analysis in mammalian cells. Proc. Natl Acad. Sci. USA 100, 12147–12152 (2003).
Conkright, M. D. et al. TORCs: Transducers of regulated CREB activity. Mol. Cell 12, 413–423 (2003).
Screaton, R. A. et al. The CREB coactivator TORC2 functions as a calcium- and cAMP-sensitive coincidence detector. Cell 119, 61–74 (2004).
Koo, S. H. et al. The CREB coactivator TORC2 is a key regulator of fasting glucose metabolism. Nature 437, 1109–1111 (2005).
Mair, W. et al. Lifespan extension induced by AMPK and calcineurin is mediated by CRTC-1 and CREB. Nature 470, 404–408 (2011).
Clark, K. et al. Phosphorylation of CRTC3 by the salt-inducible kinases controls the interconversion of classically activated and regulatory macrophages. Proc. Natl Acad. Sci. USA 109, 16986–16991 (2012).
Wu, Z. et al. Transducer of regulated CREB-binding proteins (TORCs) induce PGC-1alpha transcription and mitochondrial biogenesis in muscle cells. Proc. Natl Acad. Sci. USA 103, 14379–14384 (2006).
Than, T. A., Lou, H., Ji, C., Win, S. & Kaplowitz, N. Role of cAMP-responsive element-binding protein (CREB)-regulated transcription coactivator 3 (CRTC3) in the initiation of mitochondrial biogenesis and stress response in liver celle. J. Biol. Chem. 286, 22047–22054 (2011).
We thank Jun Wu for mouse colony maintenance and technical support, and members of the Kuang Laboratory for comments. We thank Dr Neil Kaplowitz (University of Southern California) for sharing adenovirus-shCRTC3 and control plasmids. Dr Yongxu Wang (University of Massachusetts Medical School) for the BAT cell line. Phillip Reid for assistance with video editing. The project was partially supported by funding from NIH (R01AR060652) and an incentive grant from Purdue University Office of Vice President for Research (OVPR) to S.K.
The authors declare no competing financial interests.
About this article
Cite this article
Shan, T., Xiong, Y., Zhang, P. et al. Lkb1 controls brown adipose tissue growth and thermogenesis by regulating the intracellular localization of CRTC3. Nat Commun 7, 12205 (2016). https://doi.org/10.1038/ncomms12205
Cell Death & Disease (2020)
Single‐cell RNA sequencing and lipidomics reveal cell and lipid dynamics of fat infiltration in skeletal muscle
Journal of Cachexia, Sarcopenia and Muscle (2020)
Journal of Orthopaedic Research (2020)
Frontiers in Molecular Biosciences (2020)
Animal Genetics (2020)