Diabetologia

, Volume 60, Issue 11, pp 2240–2251 | Cite as

Metabolic crosstalk between fatty pancreas and fatty liver: effects on local inflammation and insulin secretion

  • Felicia Gerst
  • Robert Wagner
  • Gabriele Kaiser
  • Madhura Panse
  • Martin Heni
  • Jürgen Machann
  • Malte N. Bongers
  • Tina Sartorius
  • Bence Sipos
  • Falko Fend
  • Christian Thiel
  • Silvio Nadalin
  • Alfred Königsrainer
  • Norbert Stefan
  • Andreas Fritsche
  • Hans-Ulrich Häring
  • Susanne Ullrich
  • Dorothea Siegel-Axel
Article

Abstract

Aims/hypothesis

Obesity-linked ectopic fat accumulation is associated with the development of type 2 diabetes. Whether pancreatic and liver steatosis impairs insulin secretion is controversial. We examined the crosstalk of human pancreatic fat cells with islets and the role of diabetogenic factors, i.e. palmitate and fetuin-A, a hepatokine released from fatty liver.

Methods

Human pancreatic resections were immunohistochemically stained for insulin, glucagon, somatostatin and the macrophage/monocyte marker CD68. Pancreatic adipocytes were identified by Oil Red O and adiponectin staining. Primary pancreatic pre-adipocytes and differentiated adipocytes were co-cultured with human islets isolated from organ donors and the metabolic crosstalk between fatty liver and fatty pancreas was mimicked by the addition of palmitate and fetuin-A. Insulin secretion was evaluated by ELISA and RIA. Cytokine expression and secretion were assessed by RT-PCR and multiplex assay, respectively. Subcellular distribution of proteins was examined by confocal microscopy and protein phosphorylation by western blotting.

Results

In human pancreatic parenchyma, highly differentiated adipocytes were detected in the proximity of islets with normal architecture and hormone distribution. Infiltration of adipocytes was associated with an increased number of CD68-positive cells within islets. In isolated primary pancreatic pre-adipocytes and differentiated adipocytes, palmitate and fetuin-A induced IL6, CXCL8 and CCL2 mRNA expression. Cytokine production was toll-like receptor 4 (TLR4)-dependent and further accentuated in pre-adipocytes when co-cultured with islets. In islets, IL6 and CXCL8 mRNA levels were also increased by fetuin-A and palmitate. Only in macrophages within the isolated islets, palmitate and fetuin-A stimulated the production of the cytotoxic cytokine IL-1β. Palmitate, but not fetuin-A, exerted pro-apoptotic effects in islet cells. Instead, fetuin-A impaired glucose-induced insulin secretion in a TLR4-independent, but c-Jun N-terminal kinase- and Ca2+-dependent, manner.

Conclusions/interpretation

These results provide the first evidence that fetuin-A-mediated metabolic crosstalk of fatty liver with islets may contribute to obesity-linked glucose blindness of beta cells, while fatty pancreas may exacerbate local inflammation.

Keywords

Adipocytes Beta cells Fetuin-A Inflammation Islets Palmitate TLR4 

Abbreviations

CT

Computed tomography

GIIS

Glucose-induced insulin secretion

hSA

human serum albumin

HU

Hounsfield units

IGI

Insulinogenic index

JNK

c-Jun N-terminal Kinase

LPS

Lipopolysaccharide

MCP-1

Monocyte chemotactic protein-1

TLR4

Toll-like receptor 4

WT

Wild-type

Introduction

The role of pancreatic steatosis in the pathogenesis of type 2 diabetes is currently under discussion and may depend on additional risk factors [1, 2, 3]. Fat accumulation in the pancreas is associated with reduced insulin secretion in glucose intolerant humans [4]. However, it is controversial whether adipocyte infiltration and altered lipid profiles of pancreatic tissue affect islet function [4, 5, 6, 7, 8].

The secretomes of fatty liver and visceral adipocytes, including the hepatokine fetuin-A and NEFA, contribute to the generation of a diabetogenic milieu [9]. These factors favour low grade tissue inflammation and insulin resistance [10, 11, 12, 13, 14]. The ultimate cause of hyperglycaemia, however, is insufficient insulin secretion as a consequence of impaired glucose-induced insulin secretion (GIIS), dedifferentiated beta cells or beta cell apoptosis [15, 16, 17, 18, 19, 20].

NEFA- and cytokine-induced beta cell death has been extensively studied [10, 21]. Multiple observations suggest that NEFA induce islet inflammation by stimulation of resident macrophages via activation of toll-like receptor 4 (TLR4) [22, 23, 24, 25]. In addition, chemokine production (i.e. monocyte chemotactic protein-1 [MCP-1] and IL-8) within islets attracts macrophages [22].

Insulin resistance in humans is associated with high levels of NEFA only in the presence of elevated plasma fetuin-A, which indicates an interaction between fetuin-A and NEFA [26, 27]. Besides its inhibitory effect on insulin receptors, fetuin-A, together with NEFA, induces inflammation in visceral adipocytes in a TLR4-dependent manner [28, 29, 30]. Recent evidence suggests that fetuin-A triggers M1 polarisation of adipose tissue macrophages [31]. However, fetuin-A, an abundant fetal serum protein, has multiple roles. As a Ca2+-binding protein it regulates Ca2+-phosphate homeostasis and calcification [32]. Fetuin-A binds NEFA and bacterial endotoxins and is a negative acute phase protein [33, 34].

Using an in vitro co-culture system of isolated human pancreatic pre-adipocytes and differentiated adipocytes with islets, we aimed to decipher potential mechanisms by which fatty liver–fatty pancreas crosstalk impairs islet function. These mechanisms may reveal the pathogenic relevance of pancreatic steatosis for glucose homeostasis in humans.

Methods

Measurements of pancreatic fat and insulin secretion in humans

Insulin sensitivity and secretion were assessed in non-diabetic participants (n = 121) using OGTTs. The anthropometric and metabolic characteristics of the cohort are shown in the electronic supplementary material (ESM) Table 1. Impaired glucose tolerance was defined as post-challenge glucose >7.8 mmol/l. Insulin secretion was assessed by the insulinogenic index (IGI; insulin30 − insulin0 [pmol/l])/(glucose30 − glucose0 [mmol/l]) or (C-peptide(0–30) [ng/ml])/(AUC glucose(0–30)). Whole body fat distribution was estimated by MRI as previously described [4, 35].

Assessment of in vivo beta cell function with the disposition index

The disposition index (IGI × insulin sensitivity index) provides a measure of beta cell function in vivo, as it takes the respective insulin sensitivity into account. An OGTT was conducted before pancreatic surgery, and blood glucose (mmol/l) and plasma insulin (pmol/l) were measured at 0, 30, 60, 90 and 120 min. The IGI was as described above. Insulin sensitivity was estimated using the Matsuda index (104/(G0×I0×(G0+G30+G60+G90+G120)/5)×( I0+I30+I60+I90+I120)/5)0.5).

Human pancreatic resections and evaluation of pancreatic steatosis

Pancreatic resections (90 individuals, age 57–75 years, BMI 22.4–27.6 kg/m2) were taken from a tumour-free region. The fat content of the whole pancreas was estimated by computed tomography (CT) in 26 participants for whom adipocyte infiltration was histologically characterised. Regions of interest were drawn in unenhanced axial slices to determine Hounsfield units (HU) in the head, body and tail of the pancreas, and the mean was calculated. A fat-free pancreas exhibits a density of 40–50 HU and adipose tissue about −90 HU.

Human islets and single cell preparation

Human islets were cultured in CMRL-1066 (ESM Table 2). For immunohistochemistry, isolated islet cells were cultured overnight on glass coverslips coated with human collagen-1 [21]. Treatment with 0.6 mg/ml human fetuin-A (Sigma-Aldrich, Munich, Germany), human serum albumin (hSA, as control) and 60 μmol/l palmitate was performed in FCS-free (to avoid exposure to bovine fetuin-A) culture medium. The concentrations of palmitate and albumin were adapted to the concentration of 0.6 mg/ml fetuin-A which matches plasma levels in glucose intolerant humans [36].

Isolation, culture and differentiation of human pancreatic pre-adipocytes

Pancreatic pre-adipocytes were isolated from adipose tissue obtained from the pancreatic resections as previously described [30]. Isolated pre-adipocytes were expanded in DMEM/Ham’s mixture F12 (1:1, ESM Table 2). FACS analysis with FITC-coupled anti-CD31 and anti-CD14 antibodies (ESM Table 3) precluded contamination with endothelial cells and monocytes/macrophages, respectively.

Adipose conversion was conducted for 7 days in DMEM/Ham’s mixture F12 (1:1, ESM Table 2). The cells were terminally differentiated for a further 7 days in medium without supplements.

Co-culture of human pancreatic fat cells and islets

Pancreatic pre-adipocytes and adipocytes were used at confluence. Human islets were placed in inserts which allows a separate analysis of fat cells and islets and media from the distinct compartments. Mono- and co-cultures were performed for 24 h in FCS-free human islet culture medium supplemented with fetuin-A, hSA and palmitate.

Gene expression

Total RNA of islets and fat cells were isolated (Nucleo Spin RNAII, Macherey-Nagel, Dueren, Germany) and transcribed using random primers (Transcriptor First Strand kits, Roche Diagnostics, Rotkreuz, Switzerland). PCR primers and probes (Light Cycler 480 System, Roche Diagnostics) are listed in ESM Table 4. Normalised gene expression was calculated as a ratio of Ct of target vs housekeeping gene (RPS13) transcripts (\( {2}^{-\Delta {\mathrm{C}}_{\mathrm{t}}} \), ΔCt), changes of expression vs control (\( {2}^{-\Delta \Delta {\mathrm{C}}_{\mathrm{t}}} \), ΔΔCt).

Cytokine and insulin quantification

Secreted cytokines were quantified using the xMAP technology (Luminex, BioRad Laboratories, Munich, Germany). Bio-Plex Pro Human Cytokine-1 5-plex EXPRESS-Kit (BioRad Laboratories) and the Human Luminex Screening Assay LXSAH-06 (R&D Systems, Minneapolis, MN, USA) were used to quantify IL-6, IL-8, MCP-1 and IL-1β proteins. Insulin was measured by RIA (Merck Millipore, Darmstadt, Germany).

Immunohistochemistry

Paraffin-embedded serial sections from 50 participants were incubated with primary antibodies (ESM Table 3). H&E was used for counterstaining. Macrophage/monocyte infiltration was quantified by counting the CD68-positive cells in islets without adipocytes in their proximity vs islets neighbouring adipocytes at a distance <400 μm. Lipids droplets were visualised using Oil Red O (0.5% in propylene glycol) after fixation of pancreatic cryosections with 4% formalin and dehydration with 100% propylene glycol.

Human islet cells were fixed with 4% formalin, permeabilised with 0.2% Triton X-100 (Sigma-Aldrich, Munich, Germany) and incubated for 1 h in 10% FCS-PBS. Primary anti-p65NFkB antibody was added overnight and secondary antibody for 1 h. Nuclei were stained with 1 μmol/l TO-PRO-3. TUNEL staining was performed according to the protocol provided with the kit (Roche Diagnostics).

Western blotting

Treated islets were lysed in RIPA buffer (ESM Table 2). Proteins were resolved using 10% SDS-PAGE and blotted onto nitrocellulose membranes. Membranes were incubated in 5% (wt/vol.) milk TBS-Tween 20 overnight with primary antibodies and for 1 h with a horse radish peroxidase-coupled secondary antibody (ESM Table 3).

Isolation, culture and insulin secretion of mouse islets

Wild-type (WT) (C57BL/6NCrl and C3H/HeNCrl) and TLR4-defective (C3H/HeJ) mouse islets were isolated using collagenase as previously described [21]. Islets were cultured in RPMI1640 (ESM Table 2). For macrophage depletion, islets were cultured for 2 days in the presence of 0.5 mg/l clodronate- or PBS (control)-containing liposomes. Afterwards, islets were cultured for 24 h or 48 h in FCS-free medium with fetuin-A, hSA and 10 μmol/l SP600125 (a c-Jun N-terminal kinase [JNK] inhibitor). Insulin secretion (10 islets/500 μl) was performed in KRB containing: 135 mmol/l NaCl, 4.8 mmol/l KCl, 1.2 mmol/l Mg2SO4, 1.2 mmol/l KH2PO4, 1.3 mmol/l CaCl2, 5 mmol/l NaHCO3, 10 mmol/l HEPES (pH 7.4), 0.5% (wt/vol.) BSA (fraction V) and glucose as indicated. Secreted insulin and insulin content after extraction with acid ethanol (1.5% (vol./vol.) HCl/75% (vol./vol.) ethanol) were measured by ELISA.

Statistics

Human tissue and cell samples were blinded before use and randomised to the treatment. Islets and islet cells were randomly distributed between the treatment groups. Statistical analysis was performed with random-intercept linear mixed models, using donors as random effects and treatments as fixed effects. The Tukey honest significant difference (HSD) test was used as post hoc test. A p value <0.05 was considered to be significant.

Study approval

All experiments with human material were approved by the Ethics Commission of the Medical Faculty and the University Hospital of the University of Tuebingen (No. 697/2011BO1 and 355/2012BO2). All participants gave informed written consent.

Isolation of mouse islets was conducted in accordance with the accepted standard of animal care and was approved by the local authorities.

Results

Negative correlation of pancreatic fat content with insulin secretion in humans

The relevance of pancreatic fat for islet function was re-evaluated in a well-defined cohort of 121 non-diabetic humans (Fig. 1a, b). While pancreatic fat content did not correlate with insulin secretion in individuals with normal glucose tolerance (Fig. 1a, β = 0.079, p = 0.38; for IGI: β = 0.068, p = 0.54) it negatively correlated with insulin secretion in humans with impaired glucose tolerance (Fig. 1b, β = −1.2, p = 0.0031; for IGI: β = −1.6, p = 0.0009). This result supports our previous observation [4].
Fig. 1

Pancreatic fat content negatively correlates with insulin secretion in humans with impaired glucose tolerance. (a, b) Association of MRI-measured pancreatic fat content with insulin secretion expressed as AUC(C-peptide)/AUC(glucose) in individuals with (a) normal glucose tolerance (β = 0.079, p = 0.38) and (b) impaired glucose tolerance (β = −1.2, p = 0.0031). Data were adjusted for insulin sensitivity using multivariate linear regression modelling. (cg) Representative pictures of human pancreatic tissue from 90 participants that were stained for (c) lipid droplets (Oil Red O) and (d) adiponectin (brown, cytosolic vesicular staining) and (eg) successive sections stained for (e) insulin, (f) glucagon and (g) somatostatin

Identification of adipocytes in human pancreatic parenchyma

Ectopic fat accumulation in the pancreas was characterised in 90 pancreatic resections. Differentiated adipocytes with a large lipid droplet and cytosolic adiponectin staining infiltrated the pancreatic tissue of 70% of the participants (Fig. 1c, d). The histological assessment of adipocyte infiltration correlated with the degree of pancreatic steatosis evaluated in the whole organ by CT measurements (ESM Fig. 1). Irrespective of the degree of adipocytes infiltration the islets displayed a normal architecture (Fig. 1e–g and ESM Fig. 2a). Most of the cells in the islet core stained for insulin, while the glucagon-containing cells were located peripherally in small and randomly in large islets, as previously reported [37]. A small number of cells stained positive for somatostatin (Fig. 1g). It is worth mentioning that even neighbouring islets displayed large variations in the proportion and distribution of glucagon-positive cells (ESM Fig. 2b).

Primary pancreatic pre-adipocytes and adipocytes are differentially stimulated by palmitate, fetuin-A and islets in co-culture

Pre-adipocytes were isolated from pancreatic adipose tissue and, following expansion, were differentiated into adipocytes (ESM Fig. 3). Adipocytes differentiation was assessed by detection of lipid droplets and ADIPOQ (encoding adiponectin) mRNA. The pre-adipocyte and adipocyte cultures were free of macrophages/monocytes, as IL-1β (IL1B) and TNF-α (TNF) were not detectable (data not shown). Under control conditions (0.6 mg/ml hSA) the pre-adipocytes and adipocytes expressed low levels of IL6 (encoding IL-6), CXCL8 (IL-8) and CCL2 (MCP-1; Fig. 2a–f, first columns). Palmitate and fetuin-A stimulated IL6, CXCL8 and CCL2 expression in pre-adipocytes and adipocytes, respectively (Fig. 2a–f). As expected, the cytokine production (IL6, CXCL8 and CCL2) was completely inhibited by the TLR4 inhibitor CLI-095 (ESM Fig. 4). Further analysis revealed that mRNA levels of TGFB1 (TGF-β1), TGFB3 (TGF-β3), VEGF and HGF remained unchanged (ESM Fig. 5).
Fig. 2

Cytokine production of pancreatic pre-adipocytes and adipocytes is stimulated by fetuin-A, palmitate and co-culture with isolated islets. (ac) Pre-adipocytes (n = 10 independent preparations) and (df) adipocytes (n = 7) were cultured for 24 h in the presence of test substances. Relative mRNA levels (ΔCt against RPS13). (gl) Pre-adipocytes were co-cultured with isolated human islets (n = 5 independent experiments) as described in the Methods. (gi) The effect of islets on pre-adipocyte mRNA levels (the fold-change [ΔΔCt] induced in pre-adipocytes by the co-culture with islets compared with mono-cultured pre-adipocytes under the same conditions, n = 5). (jl) Cytokine secretion in the pre-adipocytes compartment during mono-culture (black columns, n = 5) and co-culture (hatched columns, n = 5). Data are presented as mean ± SEM. *p < 0.05, **p < 0.01, ***p < 0.001 vs respective control (hSA); p < 0.05, ††p < 0.01, †††p < 0.001 co-culture vs mono-culture under the same conditions. Adipo, adipocytes; hFet, fetuin-A; palm, palmitate; pre-adipo, pre-adipocytes

In order to examine the paracrine crosstalk between human fat cells and islets an in vitro co-culture system was established. The co-culture with islets further increased IL6 mRNA levels of pre-adipocytes in the presence of fetuin-A, alone or with palmitate (Fig. 2g). Concurrently, CXCL8 and CCL2 mRNA levels were significantly increased by fetuin-A and palmitate (Fig. 2h, i). The rise in mRNA levels correlated with increased cytokine secretion enforcing paracrine action of pre-adipocytes on neighbouring cells (Fig. 2j–l). In contrast to the effect of islets on pre-adipocytes, cytokine production of adipocytes was not altered by islets under all co-culture conditions (data not shown).

These experiments identify the pre-adipocytes and adipocytes as highly active cell populations in the pancreatic parenchyma which secrete IL-6, IL-8 and MCP-1 upon stimulation with diabetogenic factors.

Macrophages/monocytes infiltrate islets more abundantly in proximity to adipocytes

Since fat cells produce chemo-attractants, IL-8 and MCP-1, we next analysed whether pancreatic steatosis is associated with increased local inflammation. In human pancreatic resections, a significantly higher number of CD68-positive macrophages/monocytes were found in the islets located in proximity to adipocytes (Fig. 3a–c). The mRNA analysis of laser-captured islets from pancreatic resections revealed a low expression of IL1B mRNA irrespective of the degree of pancreatic steatosis (Fig. 3d). In isolated islets from organ donors, comparable amounts of IL1B mRNA were detected (Fig. 3e, first column). Fetuin-A increased IL1B expression in isolated islets fourfold, an effect which was further augmented by the co-culture with pre-adipocytes in the presence of fetuin-A and palmitate (Fig. 3e, hatched bars).
Fig. 3

Islet macrophages/monocytes express cytotoxic cytokines. (ac) A significantly higher number of CD68-positive cells were found in islets residing in the vicinity of adipocytes. Shown are representative pictures of CD68 staining in (a) ‘adipocyte-free’ and (b) ‘fatty’ islets. The dotted boundaries in the figure enlargements mark the islet perimeter. (c) CD68-positive cell number determined in 388 ‘adipocyte-free’ (Adipos-free) and 739 ‘fatty’ (+Adipos) islets of 50 participants. (d) IL1B mRNA levels in laser-captured islets from five participants without (Adipos-free) and with (+Adipos) pancreatic steatosis. (e) IL1B mRNA levels of isolated islets mono-cultured (white bars) and co-cultured (hatched bars) with pre-adipocytes in the presence of test substances for 24 h (n = 5 independent experiments). (fh) Human islets (n = 3 independent preparations) were cultured for 48 h in the presence of PBS or clodronate liposomes (0.5 mg/ml). Thereafter, the islets were cultured for 24 h in the presence of hSA or fetuin-A. (ik) Human islets (n = 6 independent preparations) were cultured for 24 h as indicated. IL1B, CCL2, IL6 and INS mRNA levels are expressed as mean ± SEM. *p < 0.05, ***p < 0.001 vs hSA (or Adipos-free in a); †††p < 0.001 vs fetuin-A. CLI, CLI-095 (TLR4 inhibitor); Clodr-L., clodronate liposomes; hFet, fetuin-A; palm, palmitate

Upon treatment of isolated islets with clodronate liposomes which selectively depleted resident macrophages, fetuin-A-induced expression of IL1B was lost, while INS (encoding insulin) and CCL2 mRNA levels remained unchanged (Fig. 3f–h). Furthermore, inhibition of TLR4 signalling by CLI-095 (5 μmol/l) completely blocked fetuin-A-induced stimulation of IL1B and IL6 expression, whereas CCL2 mRNA levels were again not altered (Fig. 3i–k).

These observations suggest that pancreatic fat cells may accentuate macrophage/monocyte infiltration via a local production of IL-8 and MCP-1. The macrophages/monocytes, however, only secrete cytotoxic cytokines upon exposure to an adequate stimulus.

Similar to the stimulatory effect of fetuin-A and palmitate on IL6 and CXCL8 mRNA levels in fat cells, a minor but consistent increase was detectable in isolated islets (ESM Fig. 6f, g). Fetuin-A reduced SLC2A2 (encoding GLUT-2) expression, while TNF, CCL2, BLC2, TGFB1, TGFB3, VEGF and HGF mRNA levels were not altered (ESM Fig. 6). The co-culture with neither pre-adipocytes nor adipocytes affected islet mRNA levels, i.e. INS, GCG, SST, PDX1 and IRS2 (ESM Fig. 7).

Fetuin-a exerts TLR4-independent effects in islet cells

Insufficient insulin secretion during obesity is thought to result from a reduced beta cell mass due to increased beta cell apoptosis. In isolated human islet cells the apoptotic rate was enhanced by palmitate (Fig. 4a). Fetuin-A did not amplify but reversed the cytotoxic effect of palmitate. The analysis of the underlying signalling pathways suggests that, in contrast to the TLR4 agonist lipopolysaccharide (LPS), palmitate and fetuin-A, alone and together, triggered neither nuclear accumulation of NF-κB nor NF-κB phosphorylation at serine536 (Fig. 4b–e). A further indication that fetuin-A exerts TLR4-independent effects in islets was the stimulation of JNK phosphorylation in the presence of CLI-095 (Fig. 4f, g). Additional evidence for a TLR4-independent effect of fetuin-A was corroborated using TLR4-deficient mouse islets (Fig. 5). In agreement with the observation made in human islets, fetuin-A increased phosphorylation of JNK both in WT and TLR4-deficient mouse islets (Fig. 5a, b). The stimulation of JNK occurred in the absence of cytokines, since TLR4 deficiency abrogated the fetuin-A-induced increase of Il1b and Il6 mRNA levels (Fig. 5c, d).
Fig. 4

TLR4-independent effects of fetuin-A in human islet endocrine cells. (a, b) Isolated human islet cells and (cg) whole islets were cultured for (a) 24 h and (bg) 1 h as described in the Methods. (a) TUNEL staining is expressed as mean ± SEM of n = 4 independent experiments. (b) Representative pictures from three independent experiments of subcellular distribution of p65NF-κB (green); scale bar, 50 μm. Nuclei are stained in red (LPS, 1 μg/ml). (cg) Representative western blots for P-Ser536-NF-κB, NF-κB, P-Thr183/Tyr185-JNK, JNK and mean ± SEM of three independent experiments. GAPDH and tubulin were used as loading control. **p < 0.01, ***p < 0.001 vs hSA; ††p < 0.01 vs fetuin-A. CLI, CLI-095 (TLR4 inhibitor); hFet, fetuin-A; palm, palmitate

Fig. 5

Fetuin-A inhibits insulin secretion independent of TLR4. WT (C3H/HeNCrl; white bars) and TLR4-defective (C3H/HeJ; grey bars) mouse islets were cultured for (a, b) 1 h or (c, d) 24 h with test substances as indicated. (a, b) Representative western blot of P-Thr183/Tyr185-JNK and mean ± SEM of three independent experiments. (c, d) Relative mRNA levels (ΔCt) of Il1b and Il6 presented as mean ± SEM of three/four independent experiments. Insulin secretion in isolated islets from (e, f) WT (C3H/HeNCrl, white and hatched bars) and TLR4-defective (C3H/HeJ; grey and grey-hatched bars) mice after 2 days culture in the presence of hSA (white and grey bars) or fetuin-A (hatched bars). Test substances were added as indicated. Data are presented as mean ± SEM of three to five independent experiments. *p < 0.05, **p < 0.01, ***p < 0.001 vs respective hSA (bd) or respective 2.8 mmol/l glucose (e, f); p < 0.05, ††p < 0.01, †††p < 0.001 vs respective condition in WT islets (c, d) or respective hSA-cultured islets at the same condition (e, f); ‡‡‡p < 0.001 vs respective 12 mmol/l glucose. Ex-4, exendin-4 (GLP-1 analogue); Gluc, glucose; hFet, fetuin-A; palm, palmitate; SP, SP600125 (JNK inhibitor)

Next, we examined the effect of fetuin-A on insulin secretion in isolated islets from WT and TLR4-defective mice (Fig. 5e). Fetuin-A inhibited both GIIS and exendin-4-mediated augmentation of secretion in a TLR4-independent manner (Fig. 5e). When JNK was inhibited by SP600125 (10 μmol/l during 2 days of fetuin-A treatment), fetuin-A-mediated inhibition of GIIS was completely abrogated suggesting that JNK conveys the negative effect of fetuin-A on secretion (Fig. 5f).

Previously, the inhibitory effect of JNK on GIIS has been linked to a reduced glucose-induced Ca2+ influx [38]. Since fetuin-A is a Ca2+-binding protein, we examined whether an increase of the extracellular Ca2+ concentration improves GIIS of fetuin-A-treated islets. The elevation of the extracellular Ca2+ concentration from 1.3 to 2.6 mmol/l augmented GIIS and antagonised the inhibitory effect of fetuin-A in mouse islets (Fig. 6a).
Fig. 6

Increasing extracellular Ca2+ overcomes fetuin-A inhibition of insulin secretion. Isolated islets from (a) WT (C57BL/6NCrl) mice and (b) human donors were cultured for 2 days in the presence of hSA (white bars) or fetuin-A (black bars) and, thereafter, insulin secretion was stimulated with test substances as indicated. Results are expressed as mean ± SEM of three to five independent experiments, i.e. islet preparations. (c) Correlation between plasma fetuin-A and beta cell function in vivo expressed as disposition index in ten participants before surgery as described in the Methods (R2 = 0.45; p = 0.033). **p < 0.01, ***p < 0.001 vs respective secretion at 2.8 mmol/l glucose; ‡‡p < 0.01, ‡‡‡p < 0.001 vs respective secretion at 12 mmol/l glucose and 1.3 mmol/l CaCl2. Gluc, glucose; palm, palmitate

In isolated islets from human organ donors, the elevation of glucose from 2.8 to 12 mmol/l, the doubling of the concentration of extracellular CaCl2 and the addition of palmitate (600 μmol/l) significantly increased insulin secretion in control islets (Fig. 6b). In islets exposed to fetuin-A, GIIS was abrogated and the stimulatory effect of CaCl2 was significantly impaired (Fig. 6b). Palmitate-mediated stimulation of insulin secretion remained unaltered by fetuin-A. That fetuin-A affects beta cell function in vivo is further suggested by the negative correlation of plasma fetuin-A levels with the disposition index which adjusts insulin secretion for insulin sensitivity (Fig. 6c, R2 = 0.45; p = 0.033).

These results strongly suggest that fetuin-A, by stimulating JNK and interfering with the Ca2+ homeostasis, compromises glucose sensitivity of human and mouse beta cells.

Discussion

This study highlights the role of metabolic crosstalk between the pancreas and liver in the development of type 2 diabetes. Not only are the beta cells directly targeted by diabetogenic factors, i.e. palmitate and fetuin-A, but so are the pancreatic pre-adipocytes and adipocytes.

Pre-adipocytes and adipocytes contribute to pancreatic inflammation

In this study we isolated pre-adipocytes and adipocytes from human pancreatic resections and characterised their proinflammatory potential. The isolation and in vitro differentiation enabled us to identify the pre-adipocytes as further operators of tissue inflammation. Interestingly, in co-culture experiments the islets augmented the inflammatory response of pre-adipocytes. While insulin is a mandatory factor for adipocyte differentiation, local inflammation was also proposed to sustain adipogenesis [39, 40]. This could explain why highly differentiated adipocytes were detected throughout the pancreas.

Fetuin-A and palmitate induced chemokine (MCP-1 and IL-8) and cytokine (IL-6) production in human pancreatic pre-adipocytes and adipocytes. These findings reveal the fatty liver as an important player in fat cell inflammation and are in agreement with our previous studies using perivascular fat cells and the proposed proinflammatory effect of fetuin-A and palmitate via TLR4 stimulation [29, 30]. Thus, diabetes-associated factors, i.e. fetuin-A and NEFA, are putative potent activators of pancreatic fat cells.

In pancreatic resections, the adipocyte infiltration per se was not associated with altered islet architecture. Furthermore, the co-culture of islets with adipocytes and pre-adipocytes did not impair insulin secretion. In situ evaluation of CD68-positive macrophages/monocytes in pancreatic resections suggested a positive correlation between the number of macrophages/monocytes within islets and the degree of steatosis. This result suggests that the fat cells, upon stimulation by fetuin-A and palmitate, augment macrophage/monocyte infiltration via MCP-1 and IL-8. In agreement, a correlation of pancreatic steatosis with reduced insulin secretion is observed in humans with impaired glucose tolerance and fatty liver, the main source of fetuin-A and palmitate (Fig. 1 and [4, 8, 36]). Furthermore, this could be a reason why pancreatic fat is not a diabetes risk factor per se but depends on additional risk factors [3].

Fetuin-A stimulates IL-1β expression in islet-infiltrating macrophages through TLR4

It is well documented that beta cell death is triggered by cytotoxic cytokines [41, 42, 43] and may underlie the reduced beta cell mass of type 2 diabetic individuals [19, 44]. Fetuin-A stimulated IL-1β expression in islets, and the effect was mediated by TLR4. The loss of IL-1β expression in human and mouse islets depleted of macrophages strongly suggests that fetuin-A-induced inflammation is exerted on resident macrophages, not on endocrine cells. Indeed, in human pancreatic resections, CD68-positive macrophages/monocytes infiltrated the islets. In addition, we found no evidence that fetuin-A activates NF-κB in human islet cells, although a proinflammatory, TLR4-, JNK- and NF-κB-dependent effect of fetuin-A was recently ascribed to insulin secreting cells [45]. In agreement with our observations, another study identified islet resident macrophages as a source of cytokine production upon stimulation with TLR2/4 agonists [23]. Of note, fetuin-A binds LPS and NEFA with high affinity [33, 34, 46]. Although a fetuin-A preparation of high quality was used, it still contained low but detectable amounts of LPS (data not shown). Further experimental evidence is required to understand the mechanism how NEFA and LPS interact with fetuin-A to stimulate TLR4.

TLR4-independent and JNK-mediated inhibition of insulin secretion by fetuin-A

The stimulation of IL-6 production by fetuin-A was TLR4-dependent and might augment insulin secretion [47]. The use of TLR4-defective mice enabled us to dissociate the inhibitory action of fetuin-A on insulin secretion from its effects on inflammation. The inhibition of insulin secretion by fetuin-A was TLR4-independent and implied JNK activation and the impairment of cellular Ca2+ homeostasis, since it was abolished by the JNK inhibitor SP600125 and by elevation of extracellular Ca2+ concentration. Accordingly, mice with constitutively active JNK in their beta cells displayed impaired GIIS and glucose intolerance [48]. Activation of JNK may indeed inhibit insulin secretion by reduction of Ca2+ influx [38]. In agreement with our findings, fetuin-A impaired insulin secretion of the murine cell line βTC6 [45]. Clinical data showing reduced insulin secretion in humans with increased levels of fetuin-A and the negative correlation between plasma fetuin-A and the disposition index (Fig. 6c), a variable for beta cell function adjusted for insulin sensitivity, support the inhibitory effect of fetuin-A on GIIS [27, 49]. In line with a negative effect of fetuin-A on secretion, fetal islets, that are exposed to higher concentrations of fetuin-A than adult islets, are less responsive to glucose [50]. Whether a twofold increase of plasma fetuin-A concentrations – such as can be observed in individuals with hepatic steatosis – is sufficient to impair GIIS in humans remains to be clarified.

In conclusion, these results suggest that the fatty liver-derived fetuin-A impairs GIIS via a direct, TLR4-independent effect on beta cells and accentuates, in a TLR4-dependent manner, pancreatic inflammation by triggering a proinflammatory response in the pancreatic fat cells and islet macrophages/monocytes (Fig. 7). These events may accelerate beta cell failure and the progression towards overt type 2 diabetes.
Fig. 7

Fatty liver–fatty pancreas crosstalk augments pancreatic inflammation and impairs insulin secretion. (a) In the absence of fatty liver, pancreatic fat cells are in a ‘resting’ state. (b) Fatty liver-derived fetuin-A and palmitate stimulate pancreatic fat cells and islet resident macrophages. The increased expression of chemo-attractants may augment macrophage/monocyte infiltration and expression of cytotoxic proinflammatory cytokines and islet cell death. In addition, fetuin-A affects insulin secretion in a TLR4-independent manner

Notes

Acknowledgements

We would like to thank S. Wagner and L. Metzler (Department of Surgery, University Hospital Tuebingen), and L. Fritsche and A. Desseker (HMGU/IDM Tuebingen) for participant recruitment and study management. We express our gratitude to U. Schmidt and K. Bekure (HMGU/IDM Tuebingen), S. Haug, E. Metzinger and B. Schreiner (University Hospital of Tuebingen, Department of Internal Medicine IV), and B. Pömmerl (University of Tuebingen, Department of Immunology, Interfaculty institute of Cell Biology) for their skilled technical assistance.

Data availability

Data sharing not applicable to this article as no datasets were generated or analysed during the current study.

Funding

This study was supported by a grant (01GI0925) from the German Federal Ministry of Education and Research (BMBF) to the German Center for Diabetes Research (DZD e.V.). Human islets were provided by the JDRF award 31-2008-416 (ECIT Islet for Basic Research Programme) from Islet Transplantation Centres (Geneva, Milano, Lille).

Duality of interest

The authors declare that there is no duality of interest associated with this manuscript.

Contribution statement

FG, SU and DSA conceived, designed and performed experiments, analysed the data, prepared the figures and wrote the manuscript. MP and GK performed the RT-PCR experiments and analysed data. RW, MH, JM and MNB recruited and characterised participants, performed MRI and OGTT measurements, and analysed the data. AK, CT, SN, FF and BS implemented and coordinated the recruitment of participants and performed histological tissue analyses. TS implemented, managed and performed the genotyping of the mouse colony and contributed to the revision of the manuscript. NS, AF and HUH established the human cohorts, contributed to the design of the study and to the discussion of the manuscript. All authors corrected, revised and approved the final version of the manuscript. FG and SU are the guarantors of this work and, as such, had full access to all the data of the study and take responsibility for the integrity of the data and the accuracy of the data analysis.

Supplementary material

125_2017_4385_MOESM1_ESM.pdf (2.9 mb)
ESM 1(PDF 2.93 mb)

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Copyright information

© Springer-Verlag GmbH Germany 2017

Authors and Affiliations

  • Felicia Gerst
    • 1
    • 2
    • 3
  • Robert Wagner
    • 1
    • 2
    • 3
  • Gabriele Kaiser
    • 1
    • 2
    • 3
  • Madhura Panse
    • 2
    • 3
  • Martin Heni
    • 1
    • 2
    • 3
  • Jürgen Machann
    • 1
    • 2
    • 4
  • Malte N. Bongers
    • 4
  • Tina Sartorius
    • 2
    • 3
  • Bence Sipos
    • 5
  • Falko Fend
    • 5
  • Christian Thiel
    • 6
  • Silvio Nadalin
    • 6
  • Alfred Königsrainer
    • 6
  • Norbert Stefan
    • 1
    • 2
    • 3
  • Andreas Fritsche
    • 1
    • 2
    • 3
  • Hans-Ulrich Häring
    • 1
    • 2
    • 3
  • Susanne Ullrich
    • 1
    • 2
    • 3
  • Dorothea Siegel-Axel
    • 1
    • 2
    • 3
  1. 1.Institute for Diabetes Research and Metabolic Diseases of the Helmholtz Center Munich at the Eberhard Karls University of Tuebingen (IDM)TuebingenGermany
  2. 2.German Center for Diabetes Research (DZD)TuebingenGermany
  3. 3.Department of Internal Medicine IVUniversity Hospital TuebingenTuebingenGermany
  4. 4.Section of Experimental Radiology, Department of Diagnostic and Interventional RadiologyUniversity Hospital TuebingenTuebingenGermany
  5. 5.Department of General Pathology and Pathological AnatomyUniversity Hospital TuebingenTuebingenGermany
  6. 6.Department of General, Visceral and Transplant SurgeryUniversity Hospital TuebingenTuebingenGermany

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