Journal of Obesity

Journal of Obesity / 2013 / Article
Special Issue

Manifestations of Adipose Tissue Dysfunction

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Review Article | Open Access

Volume 2013 |Article ID 616193 |

Payal S. Patel, Eric D. Buras, Ashok Balasubramanyam, "The Role of the Immune System in Obesity and Insulin Resistance", Journal of Obesity, vol. 2013, Article ID 616193, 9 pages, 2013.

The Role of the Immune System in Obesity and Insulin Resistance

Academic Editor: Nicola Abate
Received29 Nov 2012
Accepted20 Feb 2013
Published21 Mar 2013


The innate immune system provides organisms with rapid and well-coordinated protection from foreign pathogens. However, under certain conditions of metabolic dysfunction, components of the innate immune system may be activated in the absence of external pathogens, leading to pathologic consequences. Indeed, there appears to be an intimate relationship between metabolic diseases and immune dysfunction; for example, macrophages are prime players in the initiation of a chronic inflammatory state in obesity which leads to insulin resistance. In response to increases in free fatty acid release from obese adipose depots, M1-polarized macrophages infiltrate adipose tissues. These M1 macrophages trigger inflammatory signaling and stress responses within cells that signal through JNK or IKKβ pathways, leading to insulin resistance. If overnutrition persists, mechanisms that counteract inflammation (such as M2 macrophages and PPAR signaling) are suppressed, and the inflammation becomes chronic. Although macrophages are a principal constituent of obese adipose tissue inflammation, other components of the immune system such as lymphocytes and mast cells also contribute to the inflammatory cascade. Thus it is not merely an increased mass of adipose tissue that directly leads to attenuation of insulin action, but rather adipose tissue inflammation activated by the immune system in obese individuals that leads to insulin resistance.

1. Introduction

The obesity epidemic in the USA continues to expand at an alarming rate, with a 75% increase in prevalence since 1980 [1]. The Centers for Disease Control and Prevention (CDC) reports that more than one-third of USA adults and over one-sixth of children and adolescents are obese. The frequencies of other metabolic disorders have increased pari passu, including dyslipidemia, nonalcoholic steatohepatitis, and type 2 diabetes. Dysfunctional adipose tissue is central to all these conditions. Adipose tissue is increasingly recognized as a complex endocrine organ and not merely a depot for storage of fat. Adipose tissue in obese persons develops an inflammatory milieu which ultimately leads to insulin resistance. Although many components of the immune system have been found to play a role in either promoting or attenuating adipose tissue inflammation, macrophages are key players. This paper discusses the various stimuli and networks that lead to insulin resistance, with a primary focus on the role of macrophages in adipose tissue inflammation.

2. Macrophage Accumulation in Visceral Adipose Tissue in Obesity

Adipose tissue comprises not only adipocytes but also a heterogenous constellation of adipocyte precursors, nerve terminals, blood vessels, and leukocytes collectively termed the “stromal vascular compartment” (SVC). In 2003, pioneering studies by Xu et al. [2] and Weisberg et al. [3] demonstrated that obesity is associated with significant increases in macrophage number within the SVC of visceral adipose tissue (VAT). Weisberg et al. discovered the increase in macrophage number through gene expression profiling of VAT from multiple obese mouse models and lean controls. They found that levels of roughly 1300 genes directly correlated with body mass, and of the 100 most significantly correlated genes, 30% were macrophage-related [3]. Detailed analysis of SVC via flow cytometry revealed that macrophages make up approximately 40% of SVC cells from obese rodents, compared to only 10% of SVC cells in lean litter mates [3].

To understand the role of macrophages in adipose tissue insulin resistance, it is important to distinguish visceral fat from subcutaneous fat. Visceral fat is found in association with internal organs such as omentum, mesentery, and perinephric adipose tissue [4]. Visceral adiposity is predictive of hepatic steatosis, cardiovascular disease, and type 2 diabetes, whereas an increase in the mass of subcutaneous fat appears to pose little or no risk of these conditions [4]. Visceral and subcutaneous fat also differ in immune cell composition, particularly macrophages [57]. Similar to mouse models, increased macrophage accumulation has been demonstrated in the adipose tissue of obese humans and those with type 2 diabetes, with significantly more macrophages residing in visceral omental fat depot compared to subcutaneous inguinal depot in these subjects [5, 6]. Additionally, while macrophage content increases in both visceral and subcutaneous fat depot following a high-fat diet (HFD) feeding, the increase is severalfold greater in VAT [4]. Overall these findings indicate that increased macrophage accumulation in VAT may be a key pathologic feature of obesity and thereby of associated conditions such as type 2 diabetes, cardiovascular disease, and fatty liver.

3. Lipolysis, Resulting in an Increase of Free Fatty Acids, Promotes Adipose Tissue Macrophage Accumulation

What is the underlying factor that promotes the accumulation of adipose tissue macrophages (ATMs)? Kosteli et al. proposed that this phenomenon may be driven by alterations in adipose metabolic function and substrate fluxes, specifically increased concentrations of free fatty acids (FFAs) [8]. They suggested that obesity causes an increase in basal lipolysis, and the resultant increase in local extracellular free fatty acid concentrations could provide a chemotactic stimulus for entry and accumulation of macrophages. Basal lipolysis is chronically elevated in adipose tissue of obese compared with lean persons and in intra-abdominal compared with subcutaneous adipose tissue [8]. Consistent with this hypothesis, visceral adipose tissue depots contain more ATMs than abdominal subcutaneous depots [8]. Many details of this process remain to be clarified. Basal lipolysis could release a number of potential signaling molecules that could play a role in macrophage chemotaxis, for example, arachidonic acid products [8]. An additional intriguing feature is that lipolysis also increases during weight loss, and ATMs recruited in response to weight loss have a more anti-inflammatory phenotype (see below) than those in the adipose tissue of stably obese animals [8]. These differences suggest that additional factors are required for the entering macrophages to take on a proinflammatory phenotype.

4. Recruitment of Macrophages in Adipose Tissue

Recruitment of macrophages into adipose tissue is an early event in obesity-induced adipose depot inflammation. However, it is only one of several early events—overnutrition also causes adipocytes to release chemokines, such as monocyte chemoattractant protein-1 (MCP-1), providing a chemotactic gradient that attracts monocytes into adipose tissue [9]; these presumably can transform into tissue resident macrophages, that is, ATMs. A variety of chemokines released from ATMs can then recruit additional monocytes/macrophages, promoting a feed-forward process [9]. For instance, MCP-1, secreted primarily by macrophages and endothelial cells, is also secreted by adipocytes [10]. The MCP-1 ligand has high affinity for C-C motif receptor 2 (CCR2) on macrophages, and signals generated by this pathway stimulate macrophage migration into inflamed or damaged tissues [10, 11]. CCR2(−/−) mice display reduced ATM content, reduced proinflammatory cytokines, and improved systemic insulin sensitivity relative to body weight-matched wild-type (WT) controls [11]. There were some confounding phenotypic changes in the CCRT(−/−) mice; however Oh et al. showed that transplanting monocytes from the CCR2(−/−) mice into WT mice or WT monocytes into MCP-1(−/−) mice also resulted in decreased ATM accumulation [12]. Similar effects were observed when obese wild-type mice were treated with a CCR2 antagonist for a short term [11]. Conversely, transgenic mice overexpressing MCP-1 in adipocytes exhibited increased ATM levels, hepatic steatosis, and insulin resistance [13].

Another critical mediator of ATM accumulation is α4 integrin, which permits macrophage adhesion to endothelial cells and their subsequent transmigration through the endothelial barrier. Mice carrying a loss-of-function α4 integrin point mutation had reduced monocyte infiltration into VWAT and were protected from obesity-induced insulin resistance [14]. Cbl-associated protein (CAP), a known regulator of glucose transport (GLUT4) in adipocytes, also promotes macrophage mobility [15]. When the CAP gene is deleted from macrophages in vivo, the knock-out (KO) mice show a decrease in ATM content with reduced tissue inflammatory markers and cytokine concentrations [16]. The chemokine LTB4 is a potent chemoattractant for neutrophils—it is mainly produced by leukocytes, but is also expressed by adipocytes, and it augments MCP-1 expression in human monocytes, thus contributing to ATM infiltration [17]. Recent studies by Spite et al. have shown that mice lacking the gene encoding the LTB4 receptor, BLT1, manifested decreased inflammation in adipose tissue and liver and were protected from systemic glucose and insulin intolerance compared to WT littermates [18]. In keeping with these findings, deletion of other monocyte chemokine receptors such as CCR5 also mitigates ATM accumulation in HFD-fed mice. CCR5 and its ligands were robustly upregulated in VWAT of HFD-induced and genetically induced obese mice [19]. However, CCR5(−/−) mice were protected from insulin resistance, glucose intolerance, and hepatic steatosis induced by HFD feeding [19]. Taken together, these findings indicate that multiple chemoattractants draw macrophages, monocytes, and neutrophils into adipose tissue. An intriguing, unstudied possibility is whether these multiple chemoattractant-receptor pairs recruit different populations of macrophages or immune cells into adipose tissues.

5. Heterogeneity of Adipose Tissue Macrophages

ATMs that reside in lean adipose tissue differ from those in obese adipose tissue. Classically activated macrophages (CAMs), termed M1, are generally stimulated by T-helper-1-type cytokines such as IFN-γ or bacterial by-products. M1 macrophages are proinflammatory, secreting cytokines such as TNF-α and IL-1β, and have high phagocytic and bactericidal potential [20]. M1 cells are generally recruited from the circulation in a CCR2-dependent manner, so it is likely that their accumulation in adipose tissues is possibly due to increased entry from the circulation. In contrast, T-helper-2-type cytokines such as interleukins (IL)-4, 10, and 13 promote alternatively activated macrophages termed M2. M2 macrophages have antiparasitic functions, secrete anti-inflammatory cytokines such as IL-10, and function in tissue repair and remodeling [21]. M2 cells are thought to be derived from replication of ATM resident macrophages—hence it is possible, but unproven, that their increase in adipose tissue is due to accelerated local multiplication (Figure 1).

Tissue macrophages respond to alterations in the local environment by changing their polarization status. Obesity not only promotes infiltration and migration of macrophages, but also induces a shift in macrophage balance towards the M1 phenotype [22]. In fact, obesity shifts the adipose M2 : M1 ratio from 4 : 1 in normal mice to 1.2 : 1 [23]. This shift is evident in the expression level of CD11c on ATMs. Macrophages are bone-marrow-derived myeloid cells; hence both M1 and M2 macrophages express the myeloid cell surface markers F4/80 and CD11b. However, only the M1 population expresses the marker CD11c, whereas M2 macrophages are CD11c(−) [24, 25]. M1, CD11c(+) recruited macrophages account for the majority of the increase in ATMs observed in obese adipose tissue, where >90% of recruited monocytes become CD11c(+) ATMs [24, 25]. Also, M1 correlates with insulin resistance as demonstrated by Patsouris et al. [26]. These investigators deleted CD11c(+) macrophages in mice using a genetic system in which the primate diphtheria toxin receptor (DTR) gene is driven by the CD11c promoter; the intention was to make CD11c(+) cells expressing DTR on their surface undergo apoptotic death when the animal was exposed to diphtheria toxin. In mice fed HFD for 16 weeks, diphtheria toxin exposure ablated about half of all ATMs, while also reducing myeloid cell content in the liver and skeletal muscle. Remarkably, only 24–48 hours after diphtheria toxin administration, glucose tolerance tests completely normalized in these mice, associated with improved insulin sensitivity in both liver and skeletal muscle [26]. This study illustrated that CD11c(+) macrophage populations (M1) are responsible for insulin resistance in obese animals and demonstrated that their continued presence is required to maintain this state.

ATM M1 polarization status is not necessarily permanent; it can revert to M2 predominance under certain circumstances. For instance, switching mice from a HFD to a chow diet [27] or treating obese mice with thiazolidinediones (TZDs) [28] changed ATM polarization from M1 to M2 and subsequently improved insulin sensitivity. Although switching HFD to chow feeding reversed adipose tissue inflammatory cytokine levels, it did not change the quantity of CD11c(+) cells until 5 weeks after the diet change, indicating that the macrophage phenotype may be dynamic [27]. Furthermore, Shaul et al. demonstrated that not all CD11c(+) cells reflect the typical M1 phenotype as defined in vitro and in conditions of acute inflammation [29]. However, to summarize current understanding of a complex and emerging paradigm of adipose inflammation, M2 predominant ATMs are typically seen in normal, lean subjects while a transformation to the M1 state propagates the inflammatory state associated with obesity.

6. Adipocyte Death and Crown-Like Structures

Macrophage accumulation in VAT occurs in the context of continuous tissue remodeling that is pathologically accelerated in the obese state. Adipocytes increase and decrease in size in order to accommodate changes in lipid load during minor fluctuations in weight. With excessive weight gain, extreme increases in adipocyte size are accompanied by an elevated frequency of adipocyte death and macrophage accumulation [30]. The accelerated adipocyte death rate could partly be explained by hypoperfusion causing an inadequate supply of oxygen in the face of expanding adipose tissue. This phenomenon of poorly oxygenated adipose tissue was first observed in mice but has also been shown in obese humans [31]. Hypoxia activates the transcription factor hypoxia-inducible factor-1α (HIF-1α), which induces expression of various target genes; deletion of HIF-1α in adipocytes partially protects mice from HFD-induced obesity and insulin resistance compared with similarly fed wild-type controls [32, 33]. Strissel et al. tracked the adipocyte death rate in obese, HFD mice by assessing VAT histology periodically for 20 weeks and found that the proportion of dead adipocytes increased from <1% of total cells to >20% during the course of the study [30]. The adipocyte death rate was associated with parallel increases in weight, numbers of ATMs (expressing CD11c), TNFα and MCP-1 levels, and insulin resistance [30].

Macrophages are not homogeneously distributed throughout VAT but rather aggregated around dead adipocytes as shown in Figure 1. Dead adipocytes lack unilocular lipid droplets and therefore do not stain for perilipin [34]. Clusters of F4/80-staining macrophages surrounding perilipin (−) adipocytes are termed “crown-like structures” (CLS) [35]. Individual CLS contain up to 15 macrophages and the majority of ATMs are localized to CLS [35]. While it is rare to see CLS in chow-fed mice, there is greater than 10-fold increase in CLS number in HFD-fed mice [36]. In genetic and HFD models of rodent obesity, CLS are more numerous in visceral compared to subcutaneous depots, and CLS number correlates directly with insulin resistance [4, 35, 36]. The same holds true in obese humans, in whom CLS are significantly enriched in omental compared to inguinal adipose tissue [5]. Furthermore, the number of omental depot CLS correlates with local levels of inflammatory mediators, insulin resistance, and systemic vascular endothelial dysfunction, in humans [5, 37]. Taken together, CLS are pathological lesions in VAT of obese subjects, and they are highly correlated with adipose inflammation and insulin resistance.

7. Inflammatory Signaling and Stress Responses Causing Insulin Resistance

Obesity-associated insulin resistance (IR) is consistently associated with elevated levels of proinflammatory cytokines such as TNFα, IL-6, and IL-1β, and neutralization of TNFα improves insulin sensitivity in obese rodents [38]. Both adipocytes and the M1 subset of ATMs are a major source of these cytokines. These cytokines activate inflammatory pathways that terminate in activation of Jun N-terminal kinase-1 (JNK1) and inhibitor of kB kinase (IKKβ), the products of which alter signaling downstream of the insulin receptor and cause insulin resistance [39, 40]. Activation of these kinases in obesity highlights the intertwined relationship of metabolic and immune pathways; JNK and IKK are the same kinases that are activated in the innate immune response, mediated by Toll-like receptor (TLR) signaling stimulated by lipopolysaccharide (LPS), peptidoglycan, double-stranded RNA, and other microbial products (Figure 2).

7.1. IKKβ Signaling Pathway

IKKβ can impact insulin signaling through at least two pathways. First, it can directly phosphorylate insulin receptor substrate protein-1 (IRS-1) on serine residues, leading to attenuation of tyrosine kinase-mediated signaling from the insulin receptor, interference of normal insulin action, and subsequent insulin resistance [39]. Secondly, IKKβ leads to phosphorylation of the inhibitor of nuclear factor-κB (IκB). In the resting unphosphorylated state, IκB forms a complex with nuclear factor-κB (NF-κB), preventing it from entering the nucleus. However, phosphorylated IκB dissociates from NF-κB and undergoes degradation; free NF-κB translocates to the nucleus, binds to DNA, and activates inflammatory mediators such as TNFα and IL-6 [41]. Arkan et al. showed that mice lacking IKKβ in myeloid cells are insulin sensitive [42]. Moreover, when these myeloid-specific IKKβ knockout mice were placed on HFDs, they became just as obese as their wild-type counterparts but were protected from obesity-induced glucose intolerance and hyperinsulinemia [42].

7.2. JNK1 Signaling Pathway

As seen in Figure 2, activation of JNK1 also results in inhibitory serine phosphorylation of IRS-1. In a manner similar to IKKβ, JNK1 can stimulate transcription of inflammatory genes in association with transcription factor activator protein 1 (AP1) [43]. Knockout (KO) of JNK1 in nonhematopoietic cells protected mice from HFD-induced insulin resistance, in part through decreased adiposity [40, 44]. By contrast, mice with JNK1 knocked out of hematopoietic cells (macrophage-specific cells) became obese on HFD, with hepatic steatosis and increased intramuscular triglyceride content, but were still protected against insulin resistance [44]. Protection against insulin resistance was conferred to these hematopoietic cell-specific KO mice by a decrease in ATM content and reduction in inflammatory pathway gene expression [44]. This experiment demonstrates that obesity and tissue lipid burden may not be sufficient to cause insulin resistance. Without the inflammatory component, obesity does not lead to appreciably impaired insulin action as demonstrated in macrophage-specific IKKβ and JNK1-KO mice [42, 44].

7.3. Toll-Like Receptors and Lipid Mediators

ATMs exist in a lipid-rich milieu, and free fatty acids, abundant in that milieu, can have a variety of effects on macrophage inflammatory pathways. For instance, omega-3 fatty acids are anti-inflammatory, polyunsaturated fatty acids are weak or neutral, and saturated fatty acids are proinflammatory [45]. Toll-like pattern recognition receptors recognize molecules that are broadly shared by pathogens. Specifically, Toll-like receptor 4 (TLR4) is expressed on macrophages and recognizes not only LPS produced by gram-negative bacteria but also saturated fatty acids; both of these ligands can activate TLR4, resulting in activation of JNK and IKKβ. TLR4 expression is increased in obesity; when the gene encoding TLR4 was deleted, HFD mice were protected from insulin resistance and weight gain compared to controls [25, 46].

Lipid species appear to regulate inflammatory signaling in macrophages through non-TLR pathways as well. Overexpression of diacylglycerol transferase-1 (DGAT-1, which catalyzes the final stage in triglyceride synthesis) in macrophages protects against adipose macrophage infiltration, inflammation, and insulin resistance [47]. This suggests that the effects of triglycerides on macrophages may not be as inimical as the effects of the precursors of triglycerides, that is, fatty acids and diacylglycerols. Diacylglycerols in particular have been implicated in insulin resistance in liver and muscle [47]. In addition, ceramides have recently been shown to activate the nucleotide-binding domain, leucine-rich-containing family, and pyrin-domain-containing (NLRP) inflammasome [48]. NLRP activation ultimately leads to IL-1β and IL-18 secretion, a response that is generally stimulated by “danger signals” of nonmicrobial origin [48]. Finally, omega-3 fatty acids have anti-inflammatory and antidiabetic effects in humans and mice. Activation of the omega-3 fatty acid receptor (GRP120) on macrophages and adipocytes reverses adipose inflammation and insulin resistance in obese mice [49].

7.4. Endoplasmic Reticulum (ER) Stress

Multiple proinflammatory sources can lead to activation of ATMs in obesity, including ER stress. ER stress can be stimulated by fatty acids, nutrient excess, improperly folded proteins, and regional areas of microhypoxia, all of which occur in obese adipose tissue. As obesity develops, protein biosynthetic pathways are upregulated, activating the unfolded protein response (UPR) in the ER [50]. The UPR comprises three main pathways controlled by ER membrane proteins: inositol-requiring enzyme (IRE)-1, protein kinase-like ER kinase (PERK), and activating transcription factor (ATF)α. All 3 branches of the UPR can directly engage inflammatory pathways through activation of IKKβ and/or JNK signaling [50]. In summary, there are numerous mechanisms propagating inflammation in obesity, but most if not all appear linked to one of two final common pathways—JNK and IKKβ—which lead to the end-result of insulin resistance.

8. Mechanisms to Counteract Inflammatory Signaling

8.1. Peroxisome Proliferator-Activated Receptors (PPARs)

PPARγ is a member of the nuclear receptor superfamily of ligand-dependent transcription factors that is predominantly expressed in adipose tissue and the intestines. PPARγ is also highly expressed in macrophages and is a natural ligand to FFAs and eicosanoids. PPARα and PPARγ function as regulators of lipid metabolism and glucose homeostasis, respectively, and are targets for fatty acid oxidizing fibrates and insulin-sensitizing TZDs, respectively [51]. As seen in Figure 2, PPAR activators inhibit the activation of inflammatory response genes by interfering with the NF-κB and AP1 signaling pathways, thereby promoting insulin sensitivity [51]. Consistent with this effect, Hevener et al. demonstrated that macrophage-specific PPARγ KO induced glucose intolerance with skeletal muscle and hepatic insulin resistance in lean mice fed a normal diet [52]. This phenotype was associated with increased expression of inflammatory markers and impaired insulin signaling in adipose tissue, muscle, and liver. Furthermore, insulin resistance became more severe in mice lacking macrophage PPARγ following HFD feeding, and these mice were only partially responsive to TZD treatment [52]. Another member of the PPAR family, PPARβ/δ, is induced by IL-4 and IL-13 to promote alternative activation of macrophages. Myeloid-specific deletion of PPARβ/δ in mice has been shown to cause insulin resistance with increased adipocyte lipolysis and severe hepatosteatosis [53]. Thus PPARs function in an anti-inflammatory manner and promote M2 polarization.

9. Other Immune Cells in Adipose Tissue Contributing to Insulin Resistance

As obesity develops, enlarging adipocytes secrete chemokines that attract immune cells. Macrophages are amongst the earliest immune cells to infiltrate adipose tissue, as their numbers increase after one week of HFD [43]. Although macrophages are vital in innate and adaptive immunity, the immune response is a result of interactions between multiple cell types. Hence, regulatory T cells, CD8+ effector T cells, B cells, mast cells, and eosinophils within adipose tissue have also been implicated in the pathogenesis of obesity-related insulin resistance.

9.1. Lymphocytes

T cells are involved in adipose tissue inflammation and IR by modifying ATM numbers and affecting polarization states. T-helper (TH) cells express the cell surface marker CD4 and comprise TH1 cells (which produce proinflammatory cytokines) and TH2 cells (which produce anti-inflammatory cytokines). Regulatory T cells (Tregs), another CD4(+) type, secrete anti-inflammatory signals, inhibit macrophage migration, and induce M2 polarization [54]. Feuerer et al. discovered that Tregs were highly enriched in the VAT of normal mice, but their numbers were strikingly reduced at this site in HFD-fed and genetically obese mice [54]. Furthermore, Treg deletion in mice induced acute elevations of TNFα and IL-6 transcripts in VAT, while inhibiting insulin signaling in muscle and liver [54]. In contrast to CD4(+) cells, T cells that express the surface antigen CD8 (known as effector or cytotoxic T cells) promote ATM accumulation and proinflammatory gene expression and are increased in number in obese adipose tissue [55]. Winer et al. highlighted the role of Tregs through analyses of T-cell deficient Rag-1(−/−) mice [56]. When placed on HFD, Rag-1(−/−) rodents were more insulin resistant than their controls. Adoptive transfer of CD4(+) to these rodents reversed the insulin resistant phenotype and abrogated VWAT inflammation; this was not observed with adoptive transfer of CD8(+) cells in Rag-1(−/−) rodents [56]. A critical unanswered question in regard to these profound effects of T cells is what in the milieu of adipose tissue activates them in the first place. It would be important to determine if the activator is a specific antigen or whether some form of completely antigen-independent T cell activation takes place.

B cells have also been ascribed functions in promoting VAT inflammation during weight gain. Winer et al. identified a VAT B-cell population that expanded with HFD feeding, with parallel increases in tissue IgM and IgG levels. Immunohistochemistry revealed deposits of these antibodies throughout VAT that mirrored the locations of CLS [57]. Mice lacking the immunoglobulin mu heavy chain (B-null mice) were protected from HFD-induced insulin resistance and displayed diminished VAT inflammation as indicated by lower numbers of M1-like macrophages and activated CD8(+) T cells. Strikingly, reconstitution of B-null mice with either wild-type (WT) B cells or serum immunoglobulins from WT HFD-fed mice was sufficient to restore the insulin resistant phenotype. Furthermore, adoptive B-cell transfer to lean WT mice induced insulin resistance [57]. These results demonstrate inflammatory pathways in which B cells and adaptive immunity play a role in insulin resistance. Again, the stimulus for B-cell activation, whether a specific antigen or otherwise, remains to be specified.

9.2. Mast Cells

Although mast cells are well known for their role in allergy and anaphylaxis, they seem to play a role in obesity as well. Altintas et al. found that subcutaneous fat of lean mice contained more mast cells, but fewer solitary macrophages and CLS than visceral fat [4]. With obesity, there was no significant change in mast cell density of subcutaneous fat, but there was a substantial increase in mast cell number in visceral fat. CLS became prevalent in visceral fat of obese mice, and their distribution paralleled that of mast cells. Immunofluorescence staining and confocal microscopy demonstrated that a subset of mast cells in adipose tissue contained and released preformed TNF-α as well [4]. In summary, subcutaneous fat differed from visceral fat by not only immune cell composition but also by having a lower prevalence of CLS both in lean and obese mice. The increase in mast cells in visceral fat of obese mice suggests a role in the pathogenesis of obesity and insulin resistance. Liu et al. discovered that in mice fed on a Western diet, genetically induced deficiency of mast cells or their pharmacological stabilization (with daily injections of disodium cromoglycate) reduces body weight gain and levels of inflammatory cytokines in serum and VAT, in conjunction with improved glucose homeostasis and energy expenditure [58].

9.3. Eosinophils

Similar to mast cells, eosinophils mediate allergic reactions in addition to combating parasites. Wu et al. demonstrated that eosinophils also participate in endorsing a M2-like ATM polarization state via IL-4 [59]. By analyzing VAT of mice on a normal chow diet, these investigators found that >90% of the IL-4-competent cells recovered were eosinophils. There was a reciprocal relationship between adipose eosinophil quantity and mouse weight. When placed on a HFD, those mice that were genetically deficient in eosinophils had increased body fat, impaired glucose tolerance, and insulin resistance in comparison to WT controls. Wu et al. also observed that mice on a HFD who were infected with helminths sustained a metabolic response characterized by decreased fasting glucose and improved insulin sensitivity from the early postinfection phase and sustained up to 35 days following infection [59].

10. Conclusion

At a histological level, adipose tissue inflammation in obesity is associated with macrophage accumulation and development of CLS. At a cellular level, the resultant insulin resistance can be explained by activation of JNK1 and IKKβ, two critical pathways mediating a range of inflammatory and stress mechanisms activated in obesity. It is interesting to note that many cellular and biochemical components of the immune system that normally protect the host from foreign pathogens, such as macrophages and TLRs, also play a pathologic role in obesity-related inflammation. Overall, adipose tissue inflammation in obesity demonstrates that the immune system and metabolism are highly integrated.


  1. K. M. Flegal, M. D. Carroll, C. L. Ogden, and C. L. Johnson, “Prevalence and trends in obesity among US adults, 1999-2000,” Journal of the American Medical Association, vol. 288, no. 14, pp. 1723–1727, 2002. View at: Google Scholar
  2. H. Xu, G. T. Barnes, Q. Yang et al., “Chronic inflammation in fat plays a crucial role in the development of obesity-related insulin resistance,” Journal of Clinical Investigation, vol. 112, no. 12, pp. 1821–1830, 2003. View at: Publisher Site | Google Scholar
  3. S. P. Weisberg, D. McCann, M. Desai, M. Rosenbaum, R. L. Leibel, and A. W. Ferrante, “Obesity is associated with macrophage accumulation in adipose tissue,” Journal of Clinical Investigation, vol. 112, no. 12, pp. 1796–1808, 2003. View at: Publisher Site | Google Scholar
  4. M. M. Altintas, A. Azad, B. Nayer et al., “Mast cells, macrophages, and crown-like structures distinguish subcutaneous from visceral fat in mice,” Journal of Lipid Research, vol. 52, no. 3, pp. 480–488, 2011. View at: Publisher Site | Google Scholar
  5. R. Cancello, J. Tordjman, C. Poitou et al., “Increased infiltration of macrophages in omental adipose tissue is associated with marked hepatic lesions in morbid human obesity,” Diabetes, vol. 55, no. 6, pp. 1554–1561, 2006. View at: Publisher Site | Google Scholar
  6. M. Kolak, J. Westerbacka, V. R. Velagapudi et al., “Adipose tissue inflammation and increased ceramide content characterize subjects with high liver fat content independent of obesity,” Diabetes, vol. 56, no. 8, pp. 1960–1968, 2007. View at: Publisher Site | Google Scholar
  7. A. Gastaldelli, Y. Miyazaki, M. Pettiti et al., “Metabolic effects of visceral fat accumulation in type 2 diabetes,” Journal of Clinical Endocrinology and Metabolism, vol. 87, no. 11, pp. 5098–5103, 2002. View at: Publisher Site | Google Scholar
  8. A. Kosteli, E. Sugaru, G. Haemmerle et al., “Weight loss and lipolysis promote a dynamic immune response in murine adipose tissue,” Journal of Clinical Investigation, vol. 120, no. 10, pp. 3466–3479, 2010. View at: Publisher Site | Google Scholar
  9. J. M. Olefsky and C. K. Glass, “Macrophages, inflammation, and insulin resistance,” Annual Review of Physiology, vol. 72, pp. 219–246, 2009. View at: Publisher Site | Google Scholar
  10. P. Wang, E. Mariman, J. Renes, and J. Keijer, “The secretory function of adipocytes in the physiology of white adipose tissue,” Journal of Cellular Physiology, vol. 216, no. 1, pp. 3–13, 2008. View at: Publisher Site | Google Scholar
  11. S. P. Weisberg, D. Hunter, R. Huber et al., “CCR2 modulates inflammatory and metabolic effects of high-fat feeding,” Journal of Clinical Investigation, vol. 116, no. 1, pp. 115–124, 2006. View at: Publisher Site | Google Scholar
  12. D. Y. Oh, H. Morinaga, S. Talukdar et al., “Increased macrophage migration into adipose tissue in obese mice,” Diabetes, vol. 61, no. 2, pp. 346–354, 2012. View at: Publisher Site | Google Scholar
  13. H. Kanda, S. Tateya, Y. Tamori et al., “MCP-1 contributes to macrophage infiltration into adipose tissue, insulin resistance, and hepatic steatosis in obesity,” Journal of Clinical Investigation, vol. 116, no. 6, pp. 1494–1505, 2006. View at: Publisher Site | Google Scholar
  14. C. C. Féral, J. G. Neels, C. Kummer, M. Slepak, J. M. Olefsky, and M. H. Ginsberg, “Blockade of α4 integrin signaling ameliorates the metabolic consequences of high-fat diet-induced obesity,” Diabetes, vol. 57, no. 7, pp. 1842–1851, 2008. View at: Publisher Site | Google Scholar
  15. L. Chang, S. H. Chiang, and A. R. Saltiel, “Insulin signaling and the regulation of glucose transport,” Molecular Medicine, vol. 10, no. 7–12, pp. 65–71, 2004. View at: Publisher Site | Google Scholar
  16. L. A. Lesniewski, S. E. Hosch, J. G. Neels et al., “Bone marrow-specific Cap gene deletion protects against high-fat diet-induced insulin resistance,” Nature Medicine, vol. 13, no. 4, pp. 455–462, 2007. View at: Publisher Site | Google Scholar
  17. S. K. Chakrabarti, Y. Wen, A. D. Dobrian et al., “Evidence for activation of inflammatory lipoxygenase pathways in visceral adipose tissue of obese Zucker rats,” American Journal of Physiology, vol. 300, no. 1, pp. E175–E187, 2011. View at: Publisher Site | Google Scholar
  18. M. Spite, J. Hellmann, Y. Tang et al., “Deficiency of the leukotriene B4 receptor, BLT-1 protects against systemic insulin resistance in diet-induced obesity,” The Journal of Immunology, vol. 187, no. 4, pp. 1942–1949, 2011. View at: Publisher Site | Google Scholar
  19. H. Kitade, K. Sawamoto, M. Nagashimada et al., “CCR5 plays a critical role in obesity-induced adipose tissue inflammation and insulin resistance by regulating both macrophage recruitment and M1/M2 status,” Diabetes, vol. 61, no. 7, pp. 1680–1690, 2012. View at: Publisher Site | Google Scholar
  20. S. Goerdt, O. Politz, K. Schledzewski et al., “Alternative versus classical activation of macrophages,” Pathobiology, vol. 67, no. 5-6, pp. 222–226, 2000. View at: Google Scholar
  21. S. Gordon, “Alternative activation of macrophages,” Nature Reviews Immunology, vol. 3, no. 1, pp. 23–35, 2003. View at: Publisher Site | Google Scholar
  22. C. N. Lumeng, J. L. Bodzin, and A. R. Saltiel, “Obesity induces a phenotypic switch in adipose tissue macrophage polarization,” Journal of Clinical Investigation, vol. 117, no. 1, pp. 175–184, 2007. View at: Publisher Site | Google Scholar
  23. C. N. Lumeng, J. B. Delproposto, D. J. Westcott, and A. R. Saltiel, “Phenotypic switching of adipose tissue macrophages with obesity is generated by spatiotemporal differences in macrophage subtypes,” Diabetes, vol. 57, no. 12, pp. 3239–3246, 2008. View at: Publisher Site | Google Scholar
  24. C. N. Lumeng, S. M. DeYoung, J. L. Bodzin, and A. R. Saltiel, “Increased inflammatory properties of adipose tissue macrophages recruited during diet-induced obesity,” Diabetes, vol. 56, no. 1, pp. 16–23, 2007. View at: Publisher Site | Google Scholar
  25. M. T. A. Nguyen, S. Favelyukis, A. K. Nguyen et al., “A subpopulation of macrophages infiltrates hypertrophic adipose tissue and is activated by free fatty acids via toll-like receptors 2 and 4 and JNK-dependent pathways,” Journal of Biological Chemistry, vol. 282, no. 48, pp. 35279–35292, 2007. View at: Publisher Site | Google Scholar
  26. D. Patsouris, P. P. Li, D. Thapar, J. Chapman, J. M. Olefsky, and J. G. Neels, “Ablation of CD11c-Positive Cells Normalizes Insulin Sensitivity in Obese Insulin Resistant Animals,” Cell Metabolism, vol. 8, no. 4, pp. 301–309, 2008. View at: Publisher Site | Google Scholar
  27. P. Li, M. Lu, M. T. Nguyen et al., “Functional heterogeneity of CD11c-positive adipose tissue macrophages in diet-induced obese mice,” The Journal of Biological Chemistry, vol. 285, no. 20, pp. 15333–15345, 2010. View at: Publisher Site | Google Scholar
  28. S. Fujisaka, I. Usui, A. Bukhari et al., “Regulatory mechanisms for adipose tissue M1 and M2 macrophages in diet-induced obese mice,” Diabetes, vol. 58, no. 11, pp. 2574–2582, 2009. View at: Publisher Site | Google Scholar
  29. M. E. Shaul, G. Bennett, K. J. Strissel, A. S. Greenberg, and M. S. Obin, “Dynamic, M2-like remodeling phenotypes of CD11c+ adipose tissue macrophages during high-fat diet—induced obesity in mice,” Diabetes, vol. 59, no. 5, pp. 1171–1181, 2010. View at: Publisher Site | Google Scholar
  30. K. J. Strissel, Z. Stancheva, H. Miyoshi et al., “Adipocyte death, adipose tissue remodeling, and obesity complications,” Diabetes, vol. 56, no. 12, pp. 2910–2918, 2007. View at: Publisher Site | Google Scholar
  31. B. Kabon, A. Nagele, D. Reddy et al., “Obesity decreases perioperative tissue oxygenation,” Anesthesiology, vol. 100, no. 2, pp. 274–280, 2004. View at: Publisher Site | Google Scholar
  32. J. Jantsch, D. Chakravortty, N. Turza et al., “Hypoxia and hypoxia-inducible factor-1α modulate lipopolysaccharide-induced dendritic cell activation and function,” Journal of Immunology, vol. 180, no. 7, pp. 4697–4705, 2008. View at: Google Scholar
  33. C. Jiang, A. Qu, T. Matsubara et al., “Disruption of hypoxia-inducible factor 1 in adipocytes improves insulin sensitivity and decreases adiposity in high-fat diet-fed mice,” Diabetes, vol. 60, no. 10, pp. 2484–2495, 2011. View at: Publisher Site | Google Scholar
  34. A. S. Greenberg, J. J. Egan, S. A. Wek, N. B. Garty, E. J. Blanchette-Mackie, and C. Londos, “Perilipin, a major hormonally regulated adipocyte-specific phosphoprotein associated with the periphery of lipid storage droplets,” Journal of Biological Chemistry, vol. 266, no. 17, pp. 11341–11346, 1991. View at: Google Scholar
  35. S. Cinti, G. Mitchell, G. Barbatelli et al., “Adipocyte death defines macrophage localization and function in adipose tissue of obese mice and humans,” Journal of Lipid Research, vol. 46, no. 11, pp. 2347–2355, 2005. View at: Publisher Site | Google Scholar
  36. I. Murano, G. Barbatelli, V. Parisani et al., “Dead adipocytes, detected as crown-like structures, are prevalent in visceral fat depots of genetically obese mice,” Journal of Lipid Research, vol. 49, no. 7, pp. 1562–1568, 2008. View at: Publisher Site | Google Scholar
  37. C. M. Apovian, S. Bigornia, M. Mott et al., “Adipose macrophage infiltration is associated with insulin resistance and vascular endothelial dysfunction in obese subjects,” Arteriosclerosis, Thrombosis, and Vascular Biology, vol. 28, no. 9, pp. 1654–1659, 2008. View at: Publisher Site | Google Scholar
  38. G. S. Hotamisligil, P. Arner, J. F. Caro, R. L. Atkinson, and B. M. Spiegelman, “Increased adipose tissue expression of tumor necrosis factor-α in human obesity and insulin resistance,” Journal of Clinical Investigation, vol. 95, no. 5, pp. 2409–2415, 1995. View at: Google Scholar
  39. Z. Gao, J. Hwang, F. Bataille et al., “Serine phosphorylation of insulin receptor substrate 1 by inhibitor κB kinase complex,” The Journal of Biological Chemistry, vol. 277, no. 50, pp. 48115–48121, 2002. View at: Publisher Site | Google Scholar
  40. J. Hirosumi, G. Tuncman, L. Chang et al., “A central role for JNK in obesity and insulin resistance,” Nature, vol. 420, no. 6913, pp. 333–336, 2002. View at: Publisher Site | Google Scholar
  41. S. Vallabhapurapu and M. Karin, “Regulation and function of NF-κB transcription factors in the immune system,” Annual Review of Immunology, vol. 27, pp. 693–733, 2009. View at: Publisher Site | Google Scholar
  42. M. C. Arkan, A. L. Hevener, F. R. Greten et al., “IKK-β links inflammation to obesity-induced insulin resistance,” Nature Medicine, vol. 11, no. 2, pp. 191–198, 2005. View at: Publisher Site | Google Scholar
  43. G. Solinas and M. Karin, “JNK1 and IKKβ: molecular links between obesity and metabolic dysfunction,” FASEB Journal, vol. 24, no. 8, pp. 2596–2611, 2010. View at: Publisher Site | Google Scholar
  44. G. Solinas, C. Vilcu, J. G. Neels et al., “JNK1 in hematopoietically derived cells contributes to diet-induced inflammation and insulin resistance without affecting obesity,” Cell Metabolism, vol. 6, no. 5, pp. 386–397, 2007. View at: Publisher Site | Google Scholar
  45. J. Y. Lee, K. H. Sohn, S. H. Rhee, and D. Hwang, “Saturated fatty acids, but not unsaturated fatty acids, induce the expression of cyclooxygenase-2 mediated through toll-like receptor 4,” Journal of Biological Chemistry, vol. 276, no. 20, pp. 16683–16689, 2001. View at: Publisher Site | Google Scholar
  46. D. M. L. Tsukumo, M. A. Carvalho-Filho, J. B. C. Carvalheira et al., “Loss-of-function mutation in toll-like receptor 4 prevents diet-induced obesity and insulin resistance,” Diabetes, vol. 56, no. 8, pp. 1986–1998, 2007. View at: Publisher Site | Google Scholar
  47. S. K. Koliwad, R. S. Streeper, M. Monetti et al., “DGAT1-dependent triacylglycerol storage by macrophages protects mice from diet-induced insulin resistance and inflammation,” Journal of Clinical Investigation, vol. 120, no. 3, pp. 756–767, 2010. View at: Publisher Site | Google Scholar
  48. B. Vandanmagsar, Y. H. Youm, A. Ravussin et al., “The NLRP3 inflammasome instigates obesity-induced inflammation and insulin resistance,” Nature Medicine, vol. 17, no. 2, pp. 179–189, 2011. View at: Publisher Site | Google Scholar
  49. A. R. Saltiel, “Fishing out a sensor for anti-inflammatory oils,” Cell, vol. 142, no. 5, pp. 672–674, 2010. View at: Publisher Site | Google Scholar
  50. S. Hummasti and G. S. Hotamisligil, “Endoplasmic reticulum stress and inflammation in obesity and diabetes,” Circulation Research, vol. 107, no. 5, pp. 579–591, 2010. View at: Publisher Site | Google Scholar
  51. V. Bocher, G. Chinetti, J. C. Fruchart, and B. Staels, “Role of the peroxisome proliferator-activated receptors (PPARS) in the regulation of lipids and inflammation control,” Journal de la Societe de Biologie, vol. 196, no. 1, pp. 47–52, 2002. View at: Google Scholar
  52. A. L. Hevener, J. M. Olefsky, D. Reichart et al., “Macrophage PPARγ is required for normal skeletal muscle and hepatic insulin sensitivity and full antidiabetic effects of thiazolidinediones,” Journal of Clinical Investigation, vol. 117, no. 6, pp. 1658–1669, 2007. View at: Publisher Site | Google Scholar
  53. K. Kang, S. M. Reilly, V. Karabacak et al., “Adipocyte-derived Th2 cytokines and myeloid PPARδ regulate macrophage polarization and insulin sensitivity,” Cell Metabolism, vol. 7, no. 6, pp. 485–495, 2008. View at: Publisher Site | Google Scholar
  54. M. Feuerer, L. Herrero, D. Cipolletta et al., “Lean, but not obese, fat is enriched for a unique population of regulatory T cells that affect metabolic parameters,” Nature Medicine, vol. 15, no. 8, pp. 930–939, 2009. View at: Publisher Site | Google Scholar
  55. S. Nishimura, I. Manabe, M. Nagasaki et al., “CD8+ effector T cells contribute to macrophage recruitment and adipose tissue inflammation in obesity,” Nature Medicine, vol. 15, no. 8, pp. 914–920, 2009. View at: Publisher Site | Google Scholar
  56. S. Winer, Y. Chan, G. Paltser et al., “Normalization of obesity-associated insulin resistance through immunotherapy,” Nature Medicine, vol. 15, no. 8, pp. 921–929, 2009. View at: Publisher Site | Google Scholar
  57. D. A. Winer, S. Winer, L. Shen et al., “B cells promote insulin resistance through modulation of T cells and production of pathogenic IgG antibodies,” Nature Medicine, vol. 17, no. 5, pp. 610–617, 2011. View at: Publisher Site | Google Scholar
  58. J. Liu, A. Divoux, J. Sun et al., “Genetic deficiency and pharmacological stabilization of mast cells reduce diet-induced obesity and diabetes in mice,” Nature Medicine, vol. 15, no. 8, pp. 940–945, 2009. View at: Publisher Site | Google Scholar
  59. D. Wu, A. B. Molofsky, H. E. Liang et al., “Eosinophils sustain adipose alternatively activated macrophages associated with glucose homeostasis,” Science, vol. 332, no. 6026, pp. 243–247, 2011. View at: Publisher Site | Google Scholar

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