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Diabetologia

, Volume 61, Issue 1, pp 182–192 | Cite as

Mouse pancreatic islet macrophages use locally released ATP to monitor beta cell activity

  • Jonathan R. Weitz
  • Madina Makhmutova
  • Joana Almaça
  • Julia Stertmann
  • Kristie Aamodt
  • Marcela Brissova
  • Stephan Speier
  • Rayner Rodriguez-DiazEmail author
  • Alejandro CaicedoEmail author
Article

Abstract

Aims/hypothesis

Tissue-resident macrophages sense the microenvironment and respond by producing signals that act locally to maintain a stable tissue state. It is now known that pancreatic islets contain their own unique resident macrophages, which have been shown to promote proliferation of the insulin-secreting beta cell. However, it is unclear how beta cells communicate with islet-resident macrophages. Here we hypothesised that islet macrophages sense changes in islet activity by detecting signals derived from beta cells.

Methods

To investigate how islet-resident macrophages respond to cues from the microenvironment, we generated mice expressing a genetically encoded Ca2+ indicator in myeloid cells. We produced living pancreatic slices from these mice and used them to monitor macrophage responses to stimulation of acinar, neural and endocrine cells.

Results

Islet-resident macrophages expressed functional purinergic receptors, making them exquisite sensors of interstitial ATP levels. Indeed, islet-resident macrophages responded selectively to ATP released locally from beta cells that were physiologically activated with high levels of glucose. Because ATP is co-released with insulin and is exclusively secreted by beta cells, the activation of purinergic receptors on resident macrophages facilitates their awareness of beta cell secretory activity.

Conclusions/interpretation

Our results indicate that islet macrophages detect ATP as a proxy signal for the activation state of beta cells. Sensing beta cell activity may allow macrophages to adjust the secretion of factors to promote a stable islet composition and size.

Keywords

ATP Beta cell Calcium imaging Macrophage Pancreas Purinergic Tissue slice 

Abbreviations

[Ca2+]i

Intracellular free Ca2+ concentration

ATPγS

Adenosine 5′-(3-thiotriphosphate)

F1

First filial generation

GABA

γ-Aminobutyric acid

GFP

Green fluorescent protein

IBA1

Ionised calcium-binding adapter molecule 1

VNUT

Vesicular nucleotide transporter

TRPV1

Transient receptor potential cation channel subfamily V member 1

Introduction

Glucose homeostasis is maintained through hormone secretion from the pancreatic islet. Insulin secretion from beta cells involves the co-release of ATP and serotonin [1, 2], which are potent stimulators of immune cells. Thus, as a by-product of hormone secretion, islet endocrine cells may activate and interact with the local population of immune cells. In response, local immune cells such as resident macrophages may provide homeostatic support. Resident macrophages in other organs (e.g. Kupffer cells, Langerhans cells, microglia) are specialised to perform tissue-specific functions needed for tissue stability [3, 4, 5]. In mice that lack islet macrophages, islets show defects in development and decreased beta cell mass [6]. The mechanisms leading to this dysfunction have not been explored, although it is now known that macrophages promote beta cell proliferation [7, 8]. These findings suggest that endocrine and immune cells interact in the islet to maintain tissue homeostasis, although the signalling mechanisms remain mostly unknown.

The role of macrophages in the islet has been studied mainly under stressful conditions (e.g. in diabetes, obesity and regeneration models) in which they contribute to inflammation and disease progression, but also promote beta cell regeneration. These studies provide information about the role of islet macrophages in the context of responses associated with inflammation and autoimmunity. By contrast, little is known about the function of the islet-resident macrophage in the normal state. Only recently have islet-resident macrophages been characterised, based on embryonic origin and on classical immunological markers [9, 10]. Resident macrophages of other tissues can sense hypoxia, hyperosmolarity, metabolic stress or extracellular matrix components to induce tissue-specific behaviours that promote local homeostasis [11]. It is still unclear, however, what aspects of the islet microenvironment are monitored by resident macrophages under normal physiological conditions.

Because macrophages exert trophic effects on beta cells [7, 8, 12], we hypothesised that to adjust the production of signals such as growth factors, islet macrophages must monitor the functional state of beta cells. Testing this hypothesis requires studying resident macrophages in a preparation in which cellular relationships are preserved. While the physiology of resident macrophages has been studied in tissue slices of organs such as the brain [13], there has not been an equivalent study of pancreas macrophages. To investigate the signals that activate islet-resident macrophages locally, we adapted a method using pancreas tissue slices for in situ imaging [14]. After confirming that the properties of pancreas macrophages remained unchanged by the slicing procedure, we conducted imaging of intracellular free Ca2+ concentration ([Ca2+]i) to determine the responses of islet-resident macrophages to stimuli activating different cell populations within the pancreas.

Methods

Mice

First filial generation (F1) mice for Ca2+ imaging experiments were bred by crossing mice that contain the fluorescent calcium indicator, GCaMP3 (Rosa-GCaMP3 mice; B6, stock no. 014538; JAX laboratories, Bar Harbor, ME, USA), with mice expressing Cre recombinase in myeloid cell-specific promoters: (LyzM)-Cre (B6, stock no. 004781; JAX laboratories); Tg(Csf1r-iCre)1Jwp (referred to herein as Csf1r-Cre; FVB, stock no. 021024; JAX laboratories); and Cx3cr1 cre mice (B6, stock no. 025524; JAX laboratories). Mice were housed in a temperature- and lighting-controlled room (lights on for 12 h). F1 offspring expressing GCaMP3 in macrophages (≥ 3 months old, both male and female) were euthanised and pancreatic tissue slices were processed as described below. All experimental protocols using mice were approved by the University of Miami Animal Care and Use Committee.

Preparation of living pancreatic tissue slices

Tissue slices were prepared from 15 young adult mice (25–30 g) as described [14]. Mice were anaesthetised with isofluorane (2% vol./vol.) and euthanised by cervical dislocation to prepare for pancreatic duct injection of low-gelling-temperature agarose (1.2% [wt/vol.], dissolved in HEPES-buffered solution as described below, without BSA; catalogue no. 39346-81-1; Sigma Aldrich, St. Louis, MO, USA). Syringes (5 ml) were filled with agarose solution, and a 30-gauge needle was used to inject in the common bile duct. After injection, tissue blocks were cut, embedded and left to solidify (4°C). Living slices were then cut (150 μm) on a vibroslicer (Leica VT1000s, Leica Biosystems, Buffalo Grove, IL, USA). Slices were incubated in HEPES-buffered solution (125 mmol/l NaCl, 5.9 mmol/l KCl, 2.56 mmol/l CaCl2, 1 mmol/l MgCl2, 25 mmol/l HEPES, 0.1% BSA [wt/vol.], pH 7.4).

Immunohistochemistry

Mice were anaesthetised, exsanguinated and perfused with 4% (wt/vol.) paraformaldehyde. Blocks of mouse pancreas (0.5 cm3) were post-fixed in 4% paraformaldehyde, cryoprotected (30% [wt/vol.] sucrose) and tissue sections (40 μm) cut on a cryostat. After permeabilisation (PBS–Triton X-100 0.3% [wt/vol.]), sections were incubated in blocking solution (Biogenex, San Ramon, CA, USA). Primary antibodies were diluted in blocking solution. To visualise macrophages, we used antibodies against ionised calcium-binding adapter molecule 1 (IBA1) (1:1000; catalogue no. 019-19741, Wako Chemicals, Richmond, VA, USA), F4/80 (1∶200, catalogue no. ab6640; Abcam, Cambridge, MA, USA) and CD206 (1∶100, catalogue no. 141721; Biolegend San Diego, CA, USA). We performed immunostaining for green fluorescent protein (GFP) (1∶200, catalogue no. ab6658; Abcam) to visualise GFP expression under the control of the myeloid promoters (see JAX laboratories mice below). Cell nuclei were stained with DAPI. Slides were mounted with ProLong Anti Fade (Invitrogen, Waltham, MA, USA). All antibodies were validated and used as per manufacturer’s instructions. See electronic supplementary materials (ESM) Methods for additional details.

Ca2+ imaging of living pancreatic tissue slices

We generated mice for [Ca2+]i imaging by using F1 mice crossed from mice expressing Cre recombinase in myeloid cell-specific promoters with mice expressing the floxed Ca2+ indicator GCaMP3 (see above). Mice (≥ 3 months old, both sexes) were euthanised, and pancreatic tissue slices were processed as described above. Living tissue slices containing GCaMP3-labelled macrophages were placed in a perfusion chamber and immersed in HEPES-buffered solution. Glucose was added to the buffered solution to give a basal glucose concentration of 3 mmol/l, unless otherwise specified. All stimuli were bath applied. Throughout the study we used the non-hydrolysable ATP agonist ATPγS (adenosine 5′-(3-thiotriphosphate; Tocris Biosciences, Bristol, UK). Antagonists were left to equilibrate with receptors for 5 min before stimulation with an agonist. For [Ca2+]i imaging, a Z-stack of ~ 15–30 confocal images was acquired every 8 s using a Leica SP5 confocal laser-scanning microscope. [Ca2+]i responses in pancreatic macrophages were quantified as the AUC of individual traces of GCaMP3 fluorescence intensity (expressed as change in fluorescence intensity compared with baseline fluorescence [ΔF/F]) during the application of stimuli. To be included in the analyses, [Ca2+]i responses had to be reproducible in three or more pancreatic slices. We further analysed and quantified pseudopodia movement and velocity using the ImageJ plugin MTrackJ (https://imagescience.org/meijering/software/mtrackj/, accessed 14 October 2016. For immunohistochemical staining after [Ca2+]i imaging, slices were processed as described in ESM Methods (Immunohistochemistry section).

Confocal imaging

Confocal images (pinhole = 1 airy unit) of randomly selected islets were acquired on a Leica SP5 confocal laser-scanning microscope with 40× magnification (NA = 0.8). Macrophages were reconstructed in Z-stacks of 15–30 confocal images (step size = 2.5–4.0 μm) and analysed using ImageJ (version 1.51 h; http://imagej.nih.gov/ij). Using confocal images, we established the location of macrophages within islets (endocrine) or in acinar regions (exocrine). Experiments were not blinded. To prevent bias, we used an automated method in ImageJ to segment different pancreas regions based on DAPI staining to determine macrophage positions.

Flow cytometry

Islet macrophages were sorted based on the viable, GFP+ and F4/80+ labelled cells. For non-macrophage internal controls, islet cells were also sorted based on the viable GFP, F4/80 population. See ESM Methods for additional details.

RT-PCR

RNA was extracted from FACS sorted islet macrophages and non-macrophage internal controls using RNeasy mini kit (Qiagen, Valencia, CA), and cDNA was prepared using the high-capacity cDNA reverse transcription kit (Applied Biosystems, Foster City, CA). cDNA products were pre-amplified 10 cycles using the TaqMan pre-amp master mix (Applied Biosystems). PCR reactions were run using TaqMan gene expression assays (Applied Biosystems) in a StepOnePlus Real-Time PCR System (Applied Biosystems).

Relative quantification of gene expression was done based on the equation relative quantification = 2−ΔCt × 1,000,000 where ΔCt is the difference between the threshold cycle (Ct) value (number of cycles at which amplification for a gene reaches a threshold) of the target gene and the threshold cycle value of the ubiquitous housekeeping gene 18s. Genes analysed: Csf1r, 18s (also known as Rn18s), Gapdh, P2rx1, P2rx2, P2rx3, P2rx4, P2rx5, P2rx6, P2rx7, P2ry1, P2ry2, P2ry4, P2ry6, P2ry10, P2ry12, P2ry13, P2ry14, Adora1, Adora2a Adora2b, Adora3.

For fold change comparisons, we used the delta delta Ct method, calculated by 2ΔΔCt. To ensure for consistent qPCR results, 18s normalised samples were compared to that of Gapdh normalised samples. Fold change differences were less than a 1.2-fold between groups when normalised to 18s vs Gapdh. Genes analysed: Csf1r, 18s, Gapdh, Tnf, Il1b, Tgfb1, Il6, Mmp2, Mmp9, Egf, Vegf (also known as Vegfa).

Data analyses and statistics

To quantify [Ca2+]i responses we calculated the AUC of the fluorescence intensity traces of GCaMP3. Our criteria for accepting [Ca2+]i responses for analyses were that responses could be elicited two or more times by the same stimulus and that the peak signal was two or more times the baseline fluctuation. Statistical comparisons were performed using Student’s t test or one-way ANOVA, followed by multiple-comparison procedures with the Tukey or Dunnett’s tests. Data are shown as means ± SEM. See ESM Methods for data analysis of immunohistochemical results.

Results

Functional responses of pancreatic macrophages in situ

To study the physiological responses of pancreatic macrophages we prepared living pancreatic slices for [Ca2+]i imaging (Fig. 1a–c). Calcium ions (Ca2+) act as second messengers in several intracellular signalling pathways that are activated by surface receptor classes, including G protein-coupled surface receptors and receptor tyrosine kinases. Increase in [Ca2+]i indicates cell activation. The role of Ca2+ in immune cell function has been shown to be biologically important and well characterised in resident macrophages such as microglia and alveolar macrophages, as well as in non-myeloid lymphocyte activity [4, 5].
Fig. 1

[Ca2+]i imaging of pancreas macrophages in situ. (a) Cre-lox model used to generate the [Ca2+]i indicator GCaMP3 under the control of myeloid-specific promoters. (b, c) Living pancreatic tissue cut using a vibroslicer (b) and placed in a recording chamber (scale bar, 100 μm) (c). Arrows denote location of pancreatic islets. (d) Confocal image of a fixed pancreatic slice from a Csf1r-Cre–GCaMP3 mouse showing GCaMP3 (green) and IBA1 (red) immunostaining, and DAPI (blue) staining of nuclei. Scale bar, 50 μm. Zoomed images of islet macrophages are also shown (scale bar, 10 μm). (e) Quantification of the proportion of IBA1-positive cells within the population of GCaMP3+ cells in slices (> 75 macrophages pooled from four sections in three mice per group). Box and whisker plot shows the median (horizontal line) with the lower and upper quartiles depicted by the bottom and top edge of the box, respectively. (f) Confocal image taken from a live video recording during [Ca2+]i imaging of macrophages in a living slice from a GCaMP3+ mouse. A maximal projection of a Z-stack of ~ 40 images is shown. The image shows islet backscatter (grey) and GCaMP3-labelled macrophages (green), with macrophages labelled 1–4. (g) Three sequential higher magnification images of macrophage ‘number 1’, shown in the dotted box in (f), showing the [Ca2+]i response to stimulation with ATP (100 μmol/l). The pseudocolour scale indicates the level of fluorescence intensity. Time points are before, during and after stimulation with ATP. Scale bar, 10 μm. (h) Traces of [Ca2+]i responses in macrophages 1–4 shown in (f). Arrows indicate time points before, during and after stimulation with ATP at which the images in (g) were taken. AU, arbitrary units

To perform [Ca2+]i imaging of macrophages in real time, we generated mouse models expressing the genetically encoded Ca2+ reporter GCaMP3 (GFP–calmodulin) selectively in myeloid cells. Using a Cre-lox system, we crossed three different strains of mice expressing Cre recombinase under myeloid-specific promoter (Csf1r-Cre, Cx3cr1 cre, [LyzM]-Cre) with floxed GCaMP3 transgenic mice (Fig. 1a). In these mouse strains, Cre expression has also been reported in dendritic cells, granulocytes and monocytes. Pancreas macrophages in Csf1r-Cre–GCaMP3 and (LyzM)-Cre–GCaMP3 mice were immunostained for the macrophage marker IBA1 and showed a high percentage (~90%) of co-localisation with GCaMP3 (Fig. 1d, e). We did not use Cx3cr1 cre–GCaMP3 mice in our functional experiments because many non-myeloid cells expressed GCaMP3 (Fig. 1e).

Isolating macrophages from their native environment can cause changes in their phenotype and does not allow study of their dynamics and interactions with the local environment in situ [15]. In contrast, by using living pancreatic slices there is minimal disruption of tissue integrity and the islet cytoarchitecture within the acinar tissue is preserved [14, 16]. We sought to establish that living tissue slices are suitable for the characterisation of the physiology of macrophages in their native environment. We found that macrophages in pancreatic tissue slices showed a morphology and cluster of differentiation (CD) profile comparable with those of macrophages in the pancreas of mice perfused with fixative (ESM Figs 1, 2) and of islet macrophages characterised using flow cytometry analysis (ESM Fig. 3). Based on these data, we conclude that the slicing procedure did not alter macrophage features.

After validating the transgenic mouse lines and the slicing procedure, we performed [Ca2+]i imaging of macrophage responses to stimuli (e.g. ESM Video). GCaMP3-expressing macrophages could be discerned both in exocrine and endocrine regions in pancreatic slices (Fig. 1f). Islets were identified based on their strong backscatter (Fig. 1f). Macrophages in endocrine and exocrine tissues responded to ATPγS (100 μmol/l) with increases in [Ca2+]i (Fig. 1g, h). After functional [Ca2+]i imaging, we immunostained pancreatic slices for macrophage markers (ESM Fig. 4). With our approach, functionally characterised macrophages, easily tracked in the immunostained slices because they retained their GCaMP3 labelling, could be further classified based on their CD profile.

Pancreatic macrophages respond selectively to beta cell-derived stimuli

Pancreatic macrophages are exposed to molecules released from acinar, neural and endocrine cells (Fig. 2a). To identify interactions between these cell types and pancreas macrophages, our strategy was to apply stimuli known to activate these cells and then monitor increases in [Ca2+]i in macrophages. To selectively stimulate beta cells, we raised the glucose concentration from 3 mmol/l to 16 mmol/l and found that this increased the frequency and amplitude of [Ca2+]i responses in macrophages (Fig. 2b, c). Cell membrane depolarisation with KCl (25 mmol/l), which stimulates endocrine cells and neurons, produced similar [Ca2+]i increases in macrophages (Fig. 2d). Macrophages in slices did not respond to application of acetylcholine (100 μmol/l), a neurotransmitter that stimulates pancreatic acinar cells and postganglionic autonomic neurons (Fig. 2f). Macrophages responded strongly to capsaicin (10 μmol/l; Fig. 2g), a stimulus for cells expressing transient receptor potential cation channel subfamily V member 1 (TRPV1) channels (e.g. visceral sensory neurons and macrophages). However, substance P (SP, 10 μmol/l), a molecule released by sensory nerves in the context of local axon reflexes [17], did not increase [Ca2+]i in macrophages.
Fig. 2

[Ca2+]i responses of pancreas macrophages to tissue-specific stimulation. (a) Diagram showing the potential inputs to pancreatic macrophages from beta cells, local autonomic neurons and pancreatic acinar cells. (b) Pancreatic macrophages in Csf1r-Cre–GCaMP3 mice displayed an increase in [Ca2+]i when the glucose concentration was increased from 3 mmol/l (3G) to 16 mmol/l (16G) (grey traces). However, not all macrophages responded (black traces). Macrophages were recorded from living pancreas slices from Csf1r-Cre–GCaMP3 mice. Dotted line represents application of 16 mmol/l glucose. (c) Quantification of [Ca2+]i responses as shown in (b), in living slices from Csf1r-Cre–GCaMP3 mice. n > 4 macrophages from three mice; *p < 0.05, Student’s t test. (d) Quantification of macrophage [Ca2+]i responses to KCl (25 mmol/l). n > 8 macrophages from three mice; *p < 0.05, Student’s t test. (e) Quantification of macrophage [Ca2+]i responses to stimulation with ATP, serotonin (5HT) or GABA. n = 4–15 macrophages, from more than three slices from two to four mice; *p < 0.05, ANOVA followed by Dunnett test for multiple comparisons with the baseline (3G). (f) Quantification of [Ca2+]i responses to acetylcholine (ACh, 25 μmol/l). n > 6 macrophages from two slices from two mice. (g) Quantification of [Ca2+]i responses to substance P (SP, 1 μmol/l) and capsaicin (Cap, 10 μmol/l). n > 9 macrophages from three slices from three mice; *p < 0.05, Student’s t test. For (cg), the average AUC is shown for [Ca2+]i responses in GCaMP3 macrophages in both endocrine and exocrine tissue. Data were also confirmed in (LyzM)-Cre–GCaMP3 mice. AU, arbitrary units

Our results suggest that pancreas macrophages responded mainly to activation of endocrine cells. We therefore examined the effects of the signalling molecules ATP, γ-aminobutyric acid (GABA) and serotonin, which are known to be released by beta cells [18, 19]. These potential paracrine signals also activate macrophages in other organs [20, 21, 22]. We observed that exposure to GABA or serotonin did not produce increases in macrophage [Ca2+]i. By contrast, ATPγS (50 μmol/l) elicited the strongest increases in [Ca2+]i (Fig. 2e).

Identification of functional purinergic receptors in pancreas macrophages

We identified ATP as a strong activator of islet and acinar macrophages (Fig. 2e). The P2 receptor antagonist suramin (20 μmol/l) blocked [Ca2+]i responses of pancreatic macrophages to ATP (Fig. 3a), confirming that purinergic receptors are involved. Macrophages in the exocrine tissue showed greater [Ca2+]i responses to low levels of ATP (10 μmol/l), while higher levels of ATP (1 mmol/l) elicited [Ca2+]i responses in endocrine and exocrine macrophages equally (Fig. 3b, c). BzATP (10 μmol/l), a P2X7 receptor agonist, ADP (10 μmol/l), a P2Y receptor agonist, MRS2693 (1 μmol/l), a nucleotide with preference for P2Y6 receptors, and MRS2768 (1 μmol/l), an agonist with preference for P2Y2 receptors, also stimulated [Ca2+]i responses in macrophages (Fig. 3d, e). The P2Y receptor agonists elicited significant increases in the [Ca2+]i responses in macrophages (Fig. 3e).
Fig. 3

Islet-resident macrophages express functional purinergic receptors. (a) Traces of [Ca2+]i responses to ATP (100 μmol/l) from Csf1r-Cre–GCaMP3 islet macrophages in pancreatic slices showing that responses were inhibited by suramin (20 μmol/l), a broad P2 receptor antagonist. (b) [Ca2+]i responses of individual macrophages to increasing concentrations of ATP in the islet (black) and exocrine regions (grey) of pancreatic slices from Csf1r-Cre–GCaMP3 mice. Vertical dotted lines denote start of 2 min stimulation. (c) Concentration–response curves for [Ca2+]i after stimulation of macrophages with ATP in islet (black circles) and exocrine regions (grey circles). Responses were quantified as AUC and were normalised as a percentage of the maximum response. n = 9 cells pooled from nine slices from four mice. (d) Traces of [Ca2+]i responses to ADP (10 μmol/l) and MRS2693 (1 μmol/l) in pancreatic slices from Csf1r-Cre–GCaMP3 mice. (e) Quantification of [Ca2+]i responses to 3 mmol/l glucose (3G), BzATP (10 μmol/l; a P2X7 receptor agonist) and the P2Y receptor agonists: ADP (10 μmol/l), MRS2768 (1 μmol/l) and MRS2693 (1 μmol/l). Data are presented as mean ± SEM. The dot plot shows the average AUC (black bar) for [Ca2+]i responses to the stimuli. n > 5 macrophages from two slices from two or three mice; *p < 0.05, ANOVA followed by Dunnett test for multiple comparisons to the baseline (3G). (f) Quantification of the mRNA levels of purinergic receptors (P2rx, P2ry and Adora) expressed by sorted islet macrophages from n = 3 independent isolations from more than three mice. Data were also confirmed in (LyzM)-Cre–GCaMP3 mice. AU, arbitrary units. Data are presented as mean ± SEM

To confirm the presence of specific purinergic receptors expressed by islet macrophages, previously identified using a physiological approach above, we performed RT-PCR on FACS-sorted macrophages from isolated islets. We found expression of mRNA for the macrophage-specific gene Csf1r, P2X receptors (P2rx4, P2rx7), P2Y receptors (P2ry2, P2ry6, p2ry14) and the P1 receptors (Adora1, Adora2a, Adora2b and Adora3; Fig. 3f). Because other cells within the islet are known to respond to ATP, we compared purinergic receptor gene expression of islet macrophages with that the F4/80 islet cell population (ESM Fig. 5). We found that most receptor genes were more highly expressed in macrophages: in particular, P2rx4 (ninefold), P2rx7 (82-fold), P2ry2 (52-fold), P2ry4 (15-fold), P2ry6 (670-fold) and the P1 receptor Adora2a (13-fold). Only the expression of Adora1, the gene for a P1 receptor known to be highly expressed in alpha cells [23], was 10.5-fold higher in the islet (F4/80) population. The results suggest that islet macrophages express high levels of purinergic receptor genes.

Acutely culturing islets with ATP alters macrophage gene expression

Pancreatic macrophages have been shown to modulate gene expression of cytokines and chemokines during diet alteration [9]. We identified functional purinergic receptors in islet macrophages and sought to identify the direct effect of acute purinergic stimulation on islet macrophage gene expression. In FACS-sorted islet macrophages, we found mRNA expression of genes encoding for matrix metalloproteinase (Mmp2) and genes characteristic of both M1 (Tnfa [also known as Tnf], Il1b) and M2 (Tgfb [Tgfb1], Il6) macrophage polarisation (Fig. 4a). Upon acute stimulation with ATP (50 μmol/l, 16 h) we found Mmp2 to be significantly downregulated when compared with the control islet culture medium (5.5 mmol/l glucose RPMI + supplements) treatment; the purinergic receptor inhibitor suramin (20 μmol/l) blocked the effect of ATP (Fig. 4b). Il6 expression was increased compared with control condition, although the change was not significant. There was no observable change in the macrophage-specific gene Csf1r (Fig. 4c) or other genes identified in the basal state (Fig. 4a). These effects were mirrored in islets acutely cultured with high glucose concentration (16 mmol/l; ESM Fig. 6), although the results were not significant.
Fig. 4

Culturing islets with ATP (16 h) alters macrophage gene expression from the basal state. (a) mRNA expression from FACS-sorted islet macrophages from Csf1r-Cre–GCaMP3 mice. ND, not detected. (bd) Changes in Mmp2, Il6 and Csf1r gene expression compared with that in control islet culture medium with and without suramin (20 μmol/l), presented as fold change. Data are presented as mean ± SEM; n = 3 independent islet preparations, with islets pooled from five mice per preparation; *p < 0.05, one-sample t test to a hypothetical value of 1

ATP induces pseudopodia movement of pancreatic macrophages

In many tissues, macrophages display characteristic movements of their fine processes to scan the microenvironment [24]. Because pancreas macrophages responded strongly to ATP, we reasoned that these increases in [Ca2+]i could lead to changes in dynamic behaviour. Therefore, in parallel with measurement of [Ca2+]i, we recorded movement of macrophage pseudopodia (Fig. 5a). Modest increases in pseudopodia movement were observed after exposure to ADP (10 μmol/l), but no observable changes in movement were seen during high glucose stimulation. Stimulation with ATP (50 μmol/l) elicited a sharp [Ca2+]i response and simultaneously increased the velocity of pseudopodia movement of macrophages (Fig. 5b, c). Thus, pancreas macrophages respond to ATP by increasing the extent and rate of microenvironment scanning. Macrophage motility, however, may not be increased by the lower levels of ATP present during physiological stimulation of beta cells.
Fig. 5

ATP stimulates movement of macrophage pseudopodia. (a) Sequential images of a Csf1r-Cre–GCaMP3-derived macrophage taken during incubation with 3 mmol/l glucose (green) and after stimulation with ATP (50 μmol/l, red). Merged image shows extended macrophage pseudopodia (red). Co-localisation of green (before ATP stimulation) and red (after ATP stimulation) staining is shown in yellow. Scale bar, 10 μm. Images were acquired at the time points denoted by the green and red arrows in (b). (b) Pancreatic macrophage Ca2+ responses to ATP (50 μmol/l; grey line) with pseudopodia process movement (black line). (c) Quantification of the velocity of macrophage processes during stimulation with 3 mmol/l glucose (3G), 16 mmol/l glucose (16G), ATP (50 μmol/l) and ADP (10 μmol/l). Macrophage pseudopodia showed increased velocity during ATP stimulation. Box and whisker plot shows the median (horizontal line) with the lower and upper quartiles depicted by the bottom and top edge of the box, respectively. n > 7 macrophages from three mice; *p < 0.05 Student’s t test. AU, arbitrary units

Pancreatic macrophages respond to endogenous ATP released from beta cells

ATP levels are generally higher inside the cell, and increased extracellular ATP generally reflects cell disruption. However, ATP can be released physiologically into the extracellular space through various mechanisms including exocytosis. In the islet microenvironment, macrophages are exposed to ATP as it is co-released with insulin from beta cells [18]. Within the mouse pancreas, islets are uniquely competent to release ATP because they express vesicular nucleotide transporter (VNUT) [25]. Concentrations of ATP can rise above 25 μmol/l around stimulated beta cells [26], matching the EC50 of the observed macrophage response to ATP (15–30 μmol/l, Fig. 3c). We therefore hypothesised that macrophages sense local changes in ATP concentration during activation of beta cells.

To test this hypothesis, we increased the glucose concentration from 3 mmol/l to 16 mmol/l and challenged the [Ca2+]i responses in macrophages with suramin (20 μmol/l). After suramin washout, activity in macrophages increased again and later subsided after return to low glucose concentrations (Fig. 6a). Suramin inhibited the increased activity during exposure to 16 mmol/l glucose quantitatively (Fig. 6b), indicating that purinergic receptors mediate the macrophage responses to beta cell activation with increased glucose concentration. By contrast, exocrine macrophages showed modest, non-significant, increases in activity during stimulation with 16 mmol/l glucose (Fig. 6c). To uncouple the direct effect of glucose on pancreatic macrophages and to pinpoint the beta cell as the source of increased spontaneous activity, we used the L-type voltage-gated Ca2+ channel blocker nifedipine, a known inhibitor of beta cell secretion [27]. Application of nifedipine (10 μmol/l) blocked [Ca2+]i responses elicited by 16 mmol/l glucose (Fig. 6d), without affecting ATP sensitivity in islet macrophages (Fig. 6e). KCl depolarisation induced increases in macrophage [Ca2+]i, but not in the presence of suramin (Fig. 6f). These results indicate that ATP released endogenously from beta cells stimulates pancreas macrophages. There was no change in macrophage [Ca2+]i response during stimulation with 16 mmol/l glucose in pancreatic slices devoid of islets (Fig. 6g, h). From these data, we propose a model for communication between pancreatic islets and their resident macrophages in which islet-resident macrophages respond to ATP and other purines released from beta cells under physiological stimulation (Fig. 6i).
Fig. 6

Pancreatic macrophages sense endogenous ATP released from insulin-secreting beta cells. (a) Spontaneous activity ([Ca2+]i responses) of pancreatic macrophages increased when beta cells were stimulated by increasing the glucose concentration from 3 mmol/l (3G) to 16 mmol/l (16G) in Csf1r-Cre-GCaMP3 mice. Grey and black traces are response traces from individual cells. Spontaneous activity was inhibited by suramin (20 μmol/l). Vertical, dotted lines denote exchange of solutions. Red dotted lines denote the start and stop of suramin (20 μmol/l) application. (b, c) Quantification of [Ca2+]i response (AUC of traces shown in a), during exposure to 3G, 16G or 16G with suramin (20 μmol/l), in macrophages from pancreatic islets (b) and from exocrine macrophages (c). n = 4–20 cells pooled from three pancreatic slices from three mice; *p < 0.05, ANOVA followed by Tukey test for multiple comparisons. (d) Activity in pancreatic macrophages induced by increasing the glucose concentration from 3G to 16G was inhibited by nifedipine (10 μmol/l). (e) Quantification of [Ca2+]i responses (AUC of traces shown in d) during exposure to 3G, 16G, 16G with nifedipine (Nife, 10 μmol/l) and 16G with ATP (50 μmol/l) and nifedipine (10 μmol/l). n = 6–12 cells pooled from three pancreatic slices from three Csf1r-Cre–GCaMP3 mice; *p < 0.05, ANOVA followed by Tukey test for multiple comparisons. (f) Quantification of [Ca2+]i responses (AUC) to exchanging solutions between 3G, KCl (25 mmol/l) and KCl (25 mmol/l) with suramin (20 μmol/l). n = 9 cells pooled from three pancreatic slices from two mice; *p < 0.05, ANOVA followed by Tukey test for multiple comparisons. (g) Spontaneous activity in pancreatic macrophages did not increase when the glucose concentration was raised from 3G to 16G in pancreatic slices devoid of islets. Macrophages became activated during stimulation with ATP (50 μmol/l). (h) Quantification of [Ca2+]i increases (AUC of traces shown in g). n = 14 cells pooled from three pancreatic slices from three mice. (i) Proposed model of macrophage communication with beta cells. Box and whisker plots show the median (horizontal line) with the lower and upper quartiles depicted by the bottom and top edge of the box, respectively. AU, arbitrary units

Discussion

Our results demonstrate that pancreatic islet macrophages express a complement of purinergic receptors that detect endogenous levels of interstitial ATP. While extracellular ATP generally reflects cell disruption, we established here that macrophages respond to ATP secreted from beta cells. ATP can therefore be considered a bona fide paracrine signal that the beta cell uses to communicate with resident macrophages.

Functional imaging in living slices allowed us to study local interactions between islet endocrine cells, local neurons, acinar cells and resident macrophages. While Ca2+ imaging of macrophages is commonly performed in other tissues [5, 28, 29], it had not been attempted in the pancreas. Immune cell infiltration and movement has been monitored in the native pancreas [30, 31, 32] but given the low spatial resolution and limited access to local drug application it is unlikely that these in vivo approaches would allow the physiological characterisation and pharmacological interrogation of macrophages in situ we conducted here.

Using our approach, we determined that islet macrophages respond to activation of endocrine cells but not to stimulation of acinar cells. Macrophage responses to endocrine cell activation with high glucose concentrations were mediated by ATP receptors. Is very likely that most of the ATP released under these conditions is derived from beta cells because: (1) beta cells of the mouse islet are the predominant cell type responding to high glucose; (2) in pancreas slices that did not contain islets, acinar macrophages did not respond to high glucose concentration; (3) beta cells release ATP from insulin granules [18, 33, 34] and (4) beta cells are the only pancreatic cells that express VNUT [25], making them uniquely competent to release stored ATP. Because ATP release is tightly coupled to insulin secretion, extracellular ATP levels can be considered a proxy for beta cell secretory activity. ATP signalling thus converts islet macrophages into local sensors of the beta cell’s hormonal output.

ATP may trigger important physiological processes in islet macrophages. Indeed, purinergic signalling has been shown to be essential for macrophage functions such as chemotaxis [35], phagocytosis [36] and cytokine production [37]. We determined that ATP induces increases in [Ca2+]i and movement of macrophage pseudopodia but the exact secretory responses triggered in islet macrophages when exposed to ATP remain unclear. Recent studies suggest that macrophages play a trophic role in beta cell proliferation but the results were obtained under extreme conditions which involved recruited macrophages [7, 8, 12].

In addition to proliferation factors, local release of proinflammatory cytokines, such as IL-1β has been shown to modulate insulin secretion [38] and is sufficient to damage human pancreatic islets [39]. IL-1β release from islet macrophages may act in a feedback loop to regulate insulin secretion. In our limited study, we did not detect significant differences in cytokine gene expression during acute treatment with ATP or high glucose. However, we did detect a significant downregulation of Mmp2. It is important to determine whether the purinergic axis between beta cells and resident macrophages regulates local inflammation (e.g. IL-1β [38]) and tissue integrity (e.g. matrix metalloproteinase 2 [40]) as well as trophic support (e.g. TGF-β [41], Il-6 [42]) during physiological and pathological states.

To fulfil their homeostatic role, macrophages must monitor the local microenvironment to detect changes in tissue characteristics, such as cell number and composition, and the acidity and osmolarity of interstitial fluids [43]. Our results suggest that resident macrophages use ATP receptors and probably TRPV1 receptors to respectively monitor beta cell activity and the acidity of the interstitial milieu in the islet. Islet macrophages have been shown to be key players in autoimmune destruction of the islet caused by type 1 diabetes [44, 45, 46, 47, 48, 49, 50, 51] and have a role in producing inflammation during type 2 diabetes [52, 53]. Here, we show that islet macrophages monitor and respond to local environmental cues not only during extreme challenges such as inflammation and autoimmunity but also during less dramatic alterations in tissue physiology. Sensing the microenvironment helps the macrophage gauge its production of factors that promote islet tissue stability.

Notes

Acknowledgements

The authors are grateful to O. Umland, the manager of the flow cytometry facility of the Diabetes Research Institute at the University of Miami, for providing expert help with flow cytometry analysis.

Data availability

All data generated or analysed during this study are included in this published article (and its supplementary files).

Funding

This work was supported by the Diabetes Research Institute Foundation and National Institutes of Health grants R56-DK-084321, R01-DK-084321, R21-ES-025673 and R01-DK111538 to AC. JS and SS were supported by the German Research Foundation (DFG)-SFB/Transregio 127 and German Ministry for Education and Research (BMBF) to the German Centre for Diabetes Research (DZD).

Duality of interest

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

Contribution statement

JRW contributed to the study’s design, collection of data and analysis and interpretation of results. JRW wrote the original draft of the manuscript. MM and JA contributed to the collection and analysis of data and critically edited the final version of the manuscript for intellectual content. JS contributed to the implementation of the pancreatic slice technique and critically edited the final version of the manuscript for intellectual content. SS contributed to the conception of the study and provided expert advice for performing the pancreatic slice and critically edited the final version of the manuscript for intellectual content. MB and KA contributed to the RT-PCR data analysis for expression of purinergic receptors and critically edited the final version of the manuscript for intellectual content. RR-D contributed to the conception of the study, collection of data and maintenance of animal colonies and critically edited the final version of the manuscript for intellectual content. AC contributed to the conception of the design of the study and data interpretation and reviewed and edited the original draft of the manuscript. AC is the guarantor of this work and has full access to the data and takes responsibility for the integrity of the work. All authors approved the final version of the manuscript.

Supplementary material

125_2017_4416_MOESM1_ESM.pdf (994 kb)
ESM (PDF 993 kb)
125_2017_4416_MOESM2_ESM.avi (1.8 mb)
ESM Video 1 (AVI 1837 kb)

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Copyright information

© Springer-Verlag GmbH Germany 2017

Authors and Affiliations

  • Jonathan R. Weitz
    • 1
    • 2
  • Madina Makhmutova
    • 1
    • 3
  • Joana Almaça
    • 1
  • Julia Stertmann
    • 4
    • 5
    • 6
  • Kristie Aamodt
    • 7
  • Marcela Brissova
    • 8
  • Stephan Speier
    • 4
    • 5
    • 6
  • Rayner Rodriguez-Diaz
    • 1
    Email author
  • Alejandro Caicedo
    • 1
    • 2
    • 3
    • 9
    Email author
  1. 1.Division of Endocrinology, Diabetes and Metabolism, Department of MedicineUniversity of Miami Miller School of MedicineMiamiUSA
  2. 2.Molecular Cell and Developmental BiologyUniversity of Miami Miller School of MedicineMiamiUSA
  3. 3.Program in NeuroscienceUniversity of Miami Miller School of MedicineMiamiUSA
  4. 4.Paul Langerhans Institute Dresden (PLID) of Helmholtz Center Munich at the University Clinic Carl Gustav Carus of Technische Universität Dresden, Helmholtz Zentrum MünchenNeuherbergGermany
  5. 5.DFG–Center for Regenerative Therapies Dresden (CRTD), Faculty of MedicineTechnische Universität DresdenDresdenGermany
  6. 6.German Center for Diabetes Research (DZD)München-NeuherbergGermany
  7. 7.Department of Molecular Physiology and BiophysicsVanderbilt University Medical CenterNashvilleUSA
  8. 8.Division of Diabetes, Endocrinology, and Metabolism, Department of MedicineVanderbilt University Medical CenterNashvilleUSA
  9. 9.Department of Physiology and Biophysics, Miller School of MedicineUniversity of MiamiMiamiUSA

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