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PLoS One. 2012; 7(4): e36368.
Published online 2012 Apr 30. doi:  10.1371/journal.pone.0036368
PMCID: PMC3340380

MFG-E8 Released by Apoptotic Endothelial Cells Triggers Anti-Inflammatory Macrophage Reprogramming

Jörg Hermann Fritz, Editor


Apoptotic endothelial cells are an important component of the “response to injury” process. Several atherosclerosis risk factors such as hyperglycemia and oxidized low-density lipoproteins, and immune injuries, such as antibodies and complement, induce endothelial cell apoptosis. While endothelial cell apoptosis is known to affect neighboring vascular wall cell biology, its consequences on macrophage reprogramming are ill defined. In this study, we report that apoptosis of human and mouse endothelial cells triggers the release of milk fat globule-epidermal growth factor 8 (MFG-E8) and reprograms macrophages into an anti-inflammatory cells. We demonstrated that MFG-E8 is released by apoptotic endothelial cells in a caspase-3-dependent manner. When macrophages were exposed to conditioned media from serum-starved apoptotic endothelial cells, they adopt a high anti-inflammatory, low pro-inflammatory cytokine/chemokine secreting phenotype that is lost if MFG-E8 is absent from the media. Macrophage treatment with recombinant MFG-E8 recapitulates the effect of conditioned media. Finally, we showed that MFG-E8-mediated reprogramming of macrophages occurs through increased phosphorylation of signal transducer and activator of transcription-3 (STAT-3). Taken together, our study suggests a key role of MFG-E8 release from apoptotic endothelial cells in macrophage reprogramming and demonstrates the importance of the apoptotic microenvironment in anti-inflammatory macrophage responses.


Apoptosis, an ubiquitous form of cell death, occurs during embryogenesis in normal tissues and during inflammation. It has been classically associated with a silent form of cell dismissal [1]. However, recent evidence suggests that apoptotic cells can modulate their microenvironment and neighboring cell biology. Apoptotic cells are known to release “eat-me” and “find-me” signals aimed at coordinating the non-phlogistic recruitment of professional phagocytes to allow swift clearance of apoptotic cells and inhibition of neutrophil influx [2], [3], [4], [5], [6], [7]. Mounting evidence indicates that the paracrine component of the apoptotic program is not limited to the regulation of leukocyte trafficking, but also prepares the cellular microenvironment for remodeling after apoptotic cell deletion. Apoptotic endothelial cells (EC) are a key component of the “response to injury” process. It is recognized that most atherosclerosis risk factors (such as hypertension [8], hyperglycemia [9] and oxidized low-density lipoproteins [10]) and antibody-complement-mediated immune injuries [11] induce EC apoptosis, which can generate a local microenvironment that will affect cell survival [12], [13], [14], [15], activation [16], [17] and differentiation [13], [18] of neighboring vascular wall cells. Apoptotic cells can modify their local environment through classical and non-classical secretion of various biological agents [15]. However, the reprogramming consequences of this apoptotic microenvironment on macrophages have not yet been fully characterized.

Macrophages are essential for initiating both inflammation and the repair of injured tissues [19]. In inflammation, they respond destructively to the damage identified; they also promote resolution of inflammation and contribute to tissue repair [20]. Initiation of inflammation, tissue damage and fibrosis are promoted by macrophages through reprogramming induced by the local microenvironment [11], [20], [21], [22], [23]. Indeed, the macrophage phenotype is affected by various signaling cues that vary according to the inflammation phase when they are recruited [20], [23]. The injury-inducing and repair-promoting role of macrophages has been well described: macrophage depletion during the fibrosis phase reduces scarring, but depletion during recovery inhibits matrix degradation [24]. Furthermore, there is evidence to suggest that macrophages have a crucial role in conditions where endothelial apoptosis is present [25], [26], [27], [28].

The local environment can affect macrophage phenotype and influence the nature of its inflammatory response. Phenotypes are dynamic; they can switch from pro-inflammatory to anti-inflammatory and vice versa [29]. Therefore, two macrophage phenotypes can be identified: pro-inflammatory (M1) and anti-inflammatory (M2). Pro-inflammatory M1 macrophages stem from classical and innate activation. They produce pro-inflammatory cytokines such as tumor necrosis factor, monocyte chemotactic protein-1 (MCP-1) and macrophage inflammatory protein-2 (MIP-2). Anti-inflammatory, pro-repair M2 macrophages derive from alternative activation or reprogramming induced by the phagocytosis of apoptotic cells. This phenotype is characterized by the production of anti-inflammatory molecules such as interleukin-10 (IL-10), transforming growth factor (TGF)-β1, and vascular endothelial growth factor (VEGF) [30], [31], [32]. However, considering phenotype as described is a simplistic view, as these macrophage phenotypes represent a continuum where transitional states are possible [33].

Our previous work, via a proteomic approach, suggested that milk fat globule-epidermal growth factor 8 (MFG-E8) could be secreted by apoptotic EC [15]. It could be produced by various cell types and, essentially, by activated macrophages. MFG-E8 is crucial for the phagocytosis of apoptotic cells [34] and in macrophage activation [35], [36]. We have further investigated MFG-E8 release by apoptotic endothelial cells due to its importance in inflammation and especially in macrophage function.

Here, we show MFG-E8 release by apoptotic EC. We propose that apoptotic EC may be the initial cellular source of MFG-E8, before its production by activated macrophages [34]. Our study suggests that apoptotic cell-conditioned media contribute to macrophage reprogramming into anti-inflammatory, pro-repair macrophages, via MFG-E8 release in a phagocytosis-independent manner.


Apoptotic endothelial cell-conditioned medium contains MFG-E8 and could program macrophages

We first assessed whether apoptotic EC could release MFG-E8. Apoptosis was induced in vitro by serum starvation (SS) for 4 h as reported previously [12], [13], [15], [37], [38]. This model is relevant to situations where EC apoptosis is found: chronic transplant vasculopathy and ischemia-reperfusion [11], [39]. In our study, serum-starved human umbilical vein endothelial cells (HUVEC) (Figure 1a), evaluated with Hoechst 33342 (HO) and propidium iodide (PI) staining, showed a progressive time-dependent increase of chromatin condensation in the absence of cell membrane permeabilization, indicative of apoptosis, as described elsewhere [12], [13], [15], [37], [38]. Necrosis, indicated by cell membrane permeabilization (inclusion of PI), was not significantly induced by SS. Chromatin condensation was present after 2 h of SS (Figure 1a), concomitantly to caspase-3 activation (Figure 1b, lower panels). Murine EC (MEC) and HUVEC apoptosis was associated with MFG-E8 release in the serum starved-conditioned media (SSC) (Figure 1b, upper panels), whereas the intracellular MFG-E8 content declined in EC, whilst simultaneously exhibiting heightened expression of active caspase-3 fragments (Figure 1b, lower panels). No significant differences were found in MFG-E8 release between BALB/c and C57BL/6 serum-starved EC (data not shown). We used mitomycin C (MMC) as another pro-apoptotic stimulus [15], [37]. MMC treatment of EC augmented the percentage of cells with chromatin condensation and promoted MFG-E8 release (Figure 1c). Furthermore, MFG-E8 was absent from media conditioned by necrotic EC suggesting that this protein is not released passively as a consequence of cell membrane permeabilization (Figure 1d). Since MFG-E8 can be secreted as a soluble or as a small membrane vesicle protein (like exosomes), we then investigated which form serum-starved EC released MFG-E8. Equal volumes of total unfractionated SSC were centrifuged at 50 000 g to remove apoptotic bodies and apoptotic cells. Supernatants and bleb pellets were collected. Obtained supernatants were then ultracentrifuged at 200 000 g to sediment small membrane vesicles, the resulting supernatants and vesicle pellets were harvested. MFG-E8 levels were detected in total unfractionated SSC, in supernatants from the centrifugation at 50 000 g and in supernatants from the 200 000 g ultracentrifugation (Figure 1e). The small membrane vesicle fraction contained MFG-E8, but at lower levels than in the supernatants. MFG-E8 was absent in the apoptotic blebs fraction (Figure 1e). These results suggest that MFG-E8 is mostly released by apoptotic EC as a soluble molecule rather than associated to small membrane vesicles.

Figure 1
Apoptotic EC-conditioned media contain MFG-E8 and reprogram macrophages.

To evaluate the phenotypic consequences of SSC on macrophage reprogramming, murine bone marrow-derived macrophages (BMDM) were stimulated with SSC for 24 h. Experiments performed with BMDM from C57BL/6 and BALB/c mice showed no differences in cytokine production between strains (data not shown). They produced more TGF-β1, VEGF and IL-10 in response to SSC from apoptotic EC than control serum-starved macrophages (Figure 1f, left panel, values in Table 1). Furthermore, the production of pro-inflammatory chemokines MCP-1 and MIP-2 was significantly lower with SSC than with SS exposure (Figure 1f, right panel, values in Table 1). Similar results were obtained with human monocytes-derived macrophages (HMDM). TGF-β1 production by HMDM was increased 2.5 times in response to SSC from apoptotic EC compared to serum starvation alone whereas production of pro-inflammatory cytokines IL-8, MCP-1 and IL-6 were 90%, 93% and 97% reduced respectively with SSC exposure compared to SS (p<0.001, n = 3). Therefore, macrophages exposed to conditioned media from serum-starved apoptotic endothelial cells, adopt a high anti-inflammatory, low pro-inflammatory cytokine/chemokine secreting phenotype.

Table 1
Phenotypic analysis of murine bone-marrow-derived macrophages exposed to SSC vs SS.

Caspase-3 activation is necessary for MFG-E8 release and subsequent macrophage programming

Employing pre-treatment with an irreversible caspase-3 specific inhibitor, DEVD (SSC-DEVD), to inhibit EC apoptosis before SS, we investigated whether MFG-E8 liberation was dependent on caspase-3 activation. As illustrated in Figure 2a (left panel), MFG-E8 release from serum-starved MEC was greatly reduced after caspase-3 inhibition using DEVD compared to control (dimethylsulfoxide (DMSO)) pre-treated serum-starved MEC (SSC-DMSO). As expected, intracellular MFG-E8 levels were higher in DEVD than in DMSO-treated MEC (Figure 2a right panel). Furthermore, serum starvation of MEC from caspase-3 knockout (KO) mice was associated with the absence of MFG-E8 release in comparison to MEC from wild type (WT) mice (Figure 2b). Moreover, MEC apoptosis plays a role in macrophage reprogramming as the anti-inflammatory phenotype of macrophages was inhibited when exposed to serum-starved MEC treated with the caspase-3 inhibitor. As depicted in Figure 2c (left panel), the production of TGF-β1, VEGF and IL-10 was significantly decreased in BMDM subjected to SSC-DEVD compared to SSC-DMSO (Figure 2c, left panel, values in Table 2). However, we observed increased MCP-1 and MIP-2 production by SSC-DEVD-treated BMDM versus the control (Figure 2c, right panel, values in Table 2). Similar results were obtained with HMDM. IL-8, MCP-1 and IL-6 production were 1.5, 2 and 10 times increased respectively in response to SSC-DEVD compared to SSC-DMSO (p<0.001, n = 3). These results suggest that caspase-3-dependent MFG-E8 production from apoptotic EC programs macrophages into an anti-inflammatory phenotype.

Figure 2
Caspase-3 activation is necessary for MFG-E8 release and subsequent macrophage reprogramming.
Table 2
Caspase-3 dependent production of MFG-E8 in EC reprograms bone-marrow-derived macrophages.

MFG-E8 plays an important and sufficient role in macrophage programming

To clearly establish that macrophage programming in response to apoptotic MEC is dependent on MFG-E8 release from apoptotic MEC, we immunoprecipitated MFG-E8 from apoptotic MEC-conditioned media. Figure 3 demonstrates that the absence of MFG-E8 significantly inhibited macrophage reprogramming by apoptotic EC. Indeed, MFG-E8-immunodepleted SSC (Figure 3, upper panel) attenuated the production of the anti-inflammatory cytokines TGF-β1, VEGF and IL-10 (Figure 3, lower left panel, values in Table 3) and increased the production of the pro-inflammatory chemokines MCP-1 and MIP-2 (Figure 3, lower right panel, values in Table 3) compared to control.

Figure 3
MFG-E8 immunoprecipitation from SSC alters macrophage reprogramming.
Table 3
Immunoprecipitation of MFG-E8 in SSC reduces the anti-inflammatory reprogramming of macrophages by SSC.

To further highlight the importance of EC-derived MFG-E8 in macrophage programming, we studied MEC derived from MFG-E8 KO mice. Immunoblotting for MFG-E8 content in supernatants and cell extracts from serum-starved KO and WT EC confirmed the absence of MFG-E8 in the KO (Figure 4a). In addition, immunoblotting revealed similar active caspase-3 levels in both KO and WT MEC (Figure 4a, right panel). SSC from MFG-E8 KO mice attenuated the production of anti-inflammatory cytokines TGF-β1 and IL-10 and increased the pro-inflammatory chemokines, MCP-1 and MIP-2, compared to SSC from MFG-E8 WT mice (Figure 4b, values in Table 4). SSC MFG-E8 KO-induced cytokine/chemokine production by macrophages was similar to that observed with the SS control (Figure 4b, values in Table 4). This suggests that the absence of MFG-E8 significantly altered macrophage programming by inducing comparable cytokine/chemokine production as seen in SS-stimulated macrophages.

Figure 4
SSC from MFG-E8 KO mice do not reprogram macrophages into anti-inflammatory macrophages.
Table 4
SSC from MFG-E8 KO mice reduces the anti-inflammatory reprogramming of macrophages.

To demonstrate the essential role of MFG-E8 in reprogramming macrophage phenotype, we performed studies with recombinant murine (rm)MFG-E8 at the same concentration as found in SSC, 1 ng/ml (data not reported). Macrophages were stimulated with rmMFG-E8 (1 ng/mL), phosphate buffered saline (PBS) (vehicle for rmMFG-E8), SS or SSC for 48 h and the supernatants were harvested. Stimulation of macrophages with rmMFG-E8 increased production of the anti-inflammatory cytokines TGF-β1, VEGF and IL-10 and decreased the production of pro-inflammatory chemokines MCP-1 and MIP-2 compared to control PBS-treated macrophages (Figure 5, values in Table 5). Chemokine/cytokine production by macrophages treated with rmMFG-E8 was similar to that seen with SSC-treated macrophages. Similar results were obtained with HMDM. TGF-β1 production by HMDM was increased by 46% in response to rhMFG-E8, whereas production of pro-inflammatory cytokines IL-8 and MCP-1 were reduced by 73% and 70% respectively with rhMFG-E8 treatment compared to control PBS-treated macrophages (p<0.001, n = 2). Taken together, these results demonstrated the importance of MFG-E8 in the induction of an anti-inflammatory macrophage phenotype.

Figure 5
Recombinant murine MFG-E8 recapitulates SSC-induced macrophage reprogramming.
Table 5
rmMFG-E8 reproduces the anti-inflammatory macrophage phenotype.

Apoptotic endothelial cell-conditioned media activated the signal transducer and activator of transcription-3 (STAT-3) pathway in macrophages

STAT family of transcription factors are involved in reprogramming of macrophages. STAT-1 activation is classically associated with the pro-inflammatory cytotoxic macrophage phenotype, whereas STAT-3 activation characterizes the pro-repair macrophages [20]. We, therefore, studied STAT-3 activation in macrophage reprogramming by apoptosis-conditioned media. Phosphorylated STAT-3 levels were higher after SSC stimulation compared to SS in BMDM (Figure 6a). We tested an experimental peritonitis model to assess the vivo reprogramming of macrophages by SSC. Pre-conditioning of peritoneal leukocytes with SSC-DMSO for 3 h increased STAT-3 phosphorylation in the cellular extracts 2 h after the induction of Brewer thioglycollate (BTG) peritonitis in mice compared to SSC-DEVD (Figure 6b, left panel). This, in turn, resulted in increased production of TGF-β1 and IL-10 (Figure 6b, right panel, see Table 6 for values). In additional studies, we determined the role of rmMFG-E8 (0.6 µg) in resident peritoneal macrophage pre-conditioning in STAT-3 activation. The administration of rmMFG-E8 increased the levels of STAT-3 phosphorylation in immunomagnetically-isolated peritoneal macrophages compared to PBS and unmanipulated control, prior to BTG injection. This STAT-3 activation persisted and increased further after BTG-induced peritonitis in isolated peritoneal macrophages compared to both controls (Figure 6c), indicating that MFG-E8 activated the STAT-3 pathway. Altogether, these results suggest that STAT-3 activation is present in the observed anti-inflammatory reprogramming of macrophages.

Figure 6
STAT-3 activation in macrophage reprogramming by apoptosis-conditioned media.
Table 6
Apoptosis-conditioned media in vivo pre-conditioning reprogram peritoneal macrophages.


Apoptotic cells release various elements that modify their microenvironment. This includes numerous chemokines or chemokine-like compounds, such as lysophosphatidylcholine [3], fractalkine [40] and nucleotides [41]. Existing evidence indicates that apoptotic EC induces resistance to apoptosis and contributes to changes in the phenotype of neighboring vascular wall cells [12], [13]. EC apoptosis, through cathepsin L release, degrades perlecan and generates the pro-fibrotic fragment LG3 [37]. Recently, other reports have suggested that the apoptotic milieu could also promote survival [14] and increase the phagocytosis of apoptotic cells by macrophages [42].

Apoptotic cells could activate classical and non-classical secretion pathways involving the exosomal release of proteins. Using proteomic analysis of media conditioned by apoptotic cells, we have previously suggested that MFG-E8 could be secreted, perhaps from the exosomal compartment [15]. However, this observation warranted further evaluation as presented here. Dendritic cells can secrete MFG-E8 through the release of exosomes [43]. Macrophages produce MFG-E8 upon activation whereas resident macrophages do not [34].

Our data highlights caspase-3-dependent MFG-E8 release by apoptotic EC as the primary source of an important protein introducing a novel mechanism of macrophage programming by the microenvironment. This apoptosis-conditioned microenvironment induces a phenotypic switch in macrophages, promoting anti-inflammatory and pro-repair macrophages, independent of apoptotic cell phagocytosis-induced reprogramming of macrophages. It suggests that, in addition to the anti-inflammatory function of apoptotic cells per se through their engulfment by macrophages and subsequent reprograming [30], [31], the apoptotic microenvironment could similarly reprogram the neighboring resident and recruited macrophages as a consequence of MFG-E8 secretion. Considering the pro-inflammatory mediators that can be produced by apoptotic EC, such as extra-cellular matrix fragments [37], a local dampening molecule could be essential to attenuate the local inflammatory response due to tissue injury. Apoptotic cells could constitute the initial source of MFG-E8 in the early inflammatory response, before production by activated macrophages [34]. The new role we are postulating for MFG-E8 could be important to maintain local tissue homeostasis by cellular death itself, to promote the pro-repair programming of macrophages and ensure the early presence of a potent apoptotic cell-opsonizing molecule [34]. This would endow MFG-E8 with another potentially crucial function. Indeed, MFG-E8 is critical for apoptotic cell phagocytosis [34] and in macrophage biology [35], [36]. During apoptotic cell engulfment, MFG-E8 opsonizes phosphatidylserine, allowing its recognition by macrophages through αvβ3 and αvβ5 integrins [34]. This process seems to occur in activated macrophages through a granulocyte-macrophage-colony-stimulating-factor induced mechanism of MFG-E8 expression [35]. In response to bacterial lipopolysaccharides (LPS) stimulation, MFG-E8 has been shown to reduce macrophage activation by modulating integrin signaling [36]. Data from an ischemia-reperfusion injury model indicates that MFG-E8 administration protects mice by promoting apoptotic cell engulfment [44]. MFG-E8 may bind lung collagen to facilitate its clearance in pulmonary fibrosis [45]. The role of MFG-E8 in inflammation extends beyond phagocytosis. Effectively, local release of TGF-β1 and CCL22 through MFG-E8 expression may foster the recruitment and maintenance of FoxP3+ Tregs, promoting allograft tolerance [35]. MFG-E8 can modify macrophage behavior by increasing IL-10 production [36]. Significantly, most of these studies have implicated macrophages as the main source of MFG-E8 production and studied its role as an inhibitor of LPS stimulation. We suggest here that apoptotic cell-conditioned media and MFG-E8 reprogram macrophages through increased STAT-3 phosphorylation. However, the signaling pathways involved in STAT-3 activation by MFG-E8 during SS are still unknown. After LPS treatment, MFG-E8 could induce STAT-3 and suppressor of cytokine signaling-3 (SOCS3) activation to attenuate the pro-inflammatory stimulation of macrophages [46]. STAT-3 has recently been implicated in MFG-E8 stimulation of cancer stem cells produced by tumor-associated macrophages [47].

In clinical situations, such as transplant vasculopathy and highly proliferative cancers, where EC apoptosis is important, the constant presence of apoptotic EC could promote an unregulated repair response by macrophages with the constant production of pro-fibrotic and immunosuppressive mediators. This could lead to tissue fibrosis and/or impaired immune response. Therefore, better understanding of MFG-E8's role in macrophage reprogramming and associated signaling pathway activated by the apoptotic cell microenvironment, is central to the development of new therapeutic approaches in transplantation and cancer biology.

Materials and Methods

Cell culture and generation of conditioned media

Human umbilical vein endothelial cells (HUVECs) (Clonetics, San Diego, CA, USA) were cultured as described elsewhere [37] and used at passages 4–5. Serum-free media conditioned by apoptotic or caspase-inhibited EC, were obtained as described (42). Equal EC numbers (2.5×104 cells/cm2) were preincubated for 2 h in normal medium containing either DMSO (vehicle) or DEVD-FMK (100 µM) (R&D Systems, Minneapolis, MN, USA) for caspase-3 inhibition, washed and the culture medium was changed for serum-free RPMI medium (Wisent, St-Bruno, Québec, Canada) and then EC were serum-starved for 4 h to obtain SSC-DMSO and SSC-DEVD respectively. To induce apoptosis in another way, EC were treated with MMC (0.01 mg/ml, Sigma, Oakville, Ontario, Canada) for 15 h. Conditioned media were collected and stored at −20°C. Conditioned media were centrifuged at 50 kG to eliminate apoptotic bodies. Necrotic conditioned media were produced by submitting EC to 3 freeze-thaw cycles. Sequential centrifugation protocol was done with 30 mL of SSC with proteases inhibitors (PMSF, Pepstatine A 2 mM, Leupeptine 2 mM), 10 mL of total SSC unfractioned was kept. 20 mL of this total SSC was then centrifuged at 50 000 g at 4°C for 15 min, blebs pellets was then resuspend in 20 mL of SS supplemented of proteases inhibitors and 10 mL were kept aside. The residual 10 mL were then ultracentrifuged at 200 000 g at 4°C for 18 h. Supernatants were kept and small membrane vesicle pellets were resuspended in 10 mL of SS supplemented with proteases inhibitors.

Murine endothelial cell (MEC) isolation

Thoracic aortae were removed surgically from anaesthetized mice, the endothelial side was placed on Matrigel (BD Bioscience, Mississauga, Ontario, Canada) for approximately a week, or until endothelial spreading was sufficient, in Dulbecco's modified Eagle's medium (DMEM) low glucose (Gibco, Burlington, Ontario, Canada) supplemented with fetal bovine serum (FBS)(Wisent, St-Bruno, Québec, Canada), calf serum (Gibco, Burlington, Ontario, Canada), endothelial cell growth supplement (VWR, Radnor, Pennsylvania, USA), heparine (Sigma, Oakville, Ontario, Canada), fugizon (Gibco, Burlington, Ontario, Canada) and penicillin/streptomycin (Wisent, St-Bruno, Québec, Canada). When the desired confluence was reached, MEC were harvested after dispase treatment and seeded on plastic flasks(BD Bioscience, Mississauga, Ontario, Canada). Cultured MEC were expanded between passages 4 and 6 and tested experimentally.

Isolation of blood monocyte-derived macrophages and preparation of bone marrow-derived macrophages

Peripheral monocytes were isolated from healthy donors by Ficoll gradient (Wisent, St-Bruno) followed by CD14+ immunomagnetic selection (Stem Cell, Vancouver). Both CD14++/CD16− and CD14low/CD16+ monocyte populations were collected. HMDM were matured in Iscove DMEM (Gibco, Burlington, Ontario, Canada) with penicillin/streptomycin (Wisent, St-Bruno, Québec, Canada), glutamine (Wisent, St-Bruno, Québec, Canada) and 10% decomplemented autologous human serum for 5–7 days before being exposed to experimental media for 24 h. Informed written consent was obtained from healthy donors according to the hospital ethics committee (comité d'éthique de la recherche du CHUM). The data were not shown. Bone marrow-derived macrophages (BMDM) were prepared from C57BL/6 mice. Bone marrow was isolated from femurs by standard sterile techniques and matured for 7 days in culture plastic in Dulbecco's modified Eagle's medium (DMEM) (Wisent, St-Bruno, Québec, Canada) with 10% FBS (Wisent, St-Bruno, Québec, Canada), penicillin/streptomycin (100 µg/ml) (Wisent, St-Bruno, Québec, Canada), and 20% L929 cell-conditioned medium as a source of macrophage-colony stimulating factor. BMDM were more than 96% positive for the macrophage marker F4/80 by flow cytometry.

Immunoblotting and reagents

In all experiments, equal volumes of all conditioned media were concentrated by centrifugation in a 10-kD vivaspin concentrator, according to the manufacturer's specifications (Sigma, Oakville, Ontario, Canada) as described previously [37] or by a trichloroacetic acid (TCA) precipitation protocol of supernatants 9∶1, washed with cold acetone and solubilization in sample buffer [15]. A fixed volume in all conditions was loaded onto gel. Proteins were separated by SDS-PAGE electrophoresis and transferred to nitrocellulose membranes. Western blotting was performed [37] and the membranes probed with anti-human MFG-E8 and anti-mouse MFG-E8 antibodies (R&D Systems, Minneapolis, MN, USA and Santa Cruz Biotechnology, Santa Cruz, CA, USA, respectively). Ponceau red staining of membranes served as protein-loading control. Proteins were extracted from cell pellets with protease or phosphatase inhibitor cocktail separated by electrophoresis, transferred to nitrocellulose or PVDF membranes, and probed. The membranes were probed with anti-active caspase-3 (Cell Signaling Technology, Pickering, Ontario, Canada), anti-β actin (Abcam, Cambridge, MA, USA), anti-phospho STAT3 and STAT3 total antibodies (Cell Signaling Technology, Pickering, Ontario, Canada).

Fluorescence microscopy for quantification of cells with chromatin condensation and cell membrane permeabilization

For fluorescence microscopy, unfixed/unpermeabilized adherent EC were stained with Hoechst 33342 (2′-(4-ethoxyphenyl)-5-(4-methyl-1-piperazinyl)-2.5′-bi-1H-benzimidazole) (HO) and PI. They were grown to confluence in 24-well culture plates (BD Bioscience, Mississauga, Ontario, Canada). HO (1 µg/ml) was added to a final concentration of 5 µg/ml immediately before fluorescence microscopy analysis (excitation filter I = 360–425 nm). Apoptotic cells show increased HO fluorescence in the absence of PI positivity. Secondary and primary necrotic cells present PI positivity.

Enzyme-linked immunosorbent assay (ELISA)

Human IL-6, -8, active TGF-β1, MCP-1 protein levels, as well as murine IL-10, MCP-1, macrophage inflammatory protein-2 (MIP-2) and vascular endothelial growth factor (VEGF) were measured by ELISA) according to the supplier's protocol (BD Bioscience, Mississauga, Ontario, Canada and R&D Systems, Minneapolis, MN, USA).

MFG-E8 immunoprecipitation from MEC and HUVEC SSC

SSC were incubated with specific antibodies against MFG-E8 or control antibody for 6 h. Protein A/G linked beads were incubated overnight at 4°C under agitation. SSC were then centrifuged and immunoblotted for MFG-E8 (Santa Cruz Biotechnology, Santa Cruz, CA, USA).

Recombinant murine MFG-E8

BMDM matured for 7 days were stimulated with rmMFG-E8 (R&D Systems, Minneapolis, MN, USA) 1 ng/mL in serum-free media (Wisent, St-Bruno, Québec, Canada) for 48 h. PBS added to serum-free media (Wisent, St-Bruno, Québec, Canada) served as negative control. Cytokines/chemokines from the supernatants were evaluated by ELISA.

Experimental animals and induction of experimental peritonitis

C57BL/6 and BALB/c mice were bought from Charles River (Canada). We acquired the MFG-E8 KO mice on the C57BL/6 background were generously donated to us by Professor S. Nagata. Caspase-3 KO mice were obtained from Jackson Laboratory. Mice were housed in CRCHUM animal facilities. They were injected intraperitoneally (IP) with 0.5 mL of conditioned media or rmMFG-E8 (0.6 µg) for 3 h and then injected with 3% Brewer's thioglycollate (BTG) (Difco) and underwent peritoneal lavage with 5 mL of phosphate buffered saline (PBS) (Wisent, St-Bruno, Québec, Canada) at 2 h thereafter. Peritoneal lavage fluid was centrifuged and stored at −80°C until analyzed for cytokine/chemokine production by ELISA. Macrophages were immunomagnetically-isolated with magnetic beads (Miltenyi Biotech, Auburn, CA, USA) after the peritoneal lavages and kept for immunoblotting. Performed animal experiments were approved by our institutional Animal Care Committee (Comité institutionnel de protection des animaux, CRCHUM).

Statistical analysis

The results are expressed as mean ± SD were analyzed by Student's T-test (with Bonferroni correction when appropriate) or ANOVA, as appropriate. p<0.05 was deemed to be significant for all tests.


We would like to thank Mrs. M. Soulez for her help with the EC culture and Mr. O. Da Silva for editing this manuscript.


Competing Interests: The authors have declared that no competing interests exist.

Funding: This work was funded in part by research grants from the Kidney Foundation of Canada, the Fonds de la recherche en santé du Québec (FRSQ), the Foundation from the Centre hospitalier de l'Université de Montréal (CHUM), and from l'Institut du Cancer de Montréal. JFC was the recipient of a Kidney Foundation of Canada scholarship and is now a FRSQ clinician-scientist scholar. The authors thank the J.-L. Lévesque Foundation and the CHUM Renal Division for their support. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.


1. Savill J, Dransfield I, Gregory C, Haslett C. A blast from the past: clearance of apoptotic cells regulates immune responses. Nat Rev Immunol. 2002;2:965–975. [PubMed]
2. Schaub FJ, Han DK, Liles WC, Adams LD, Coats SA, et al. Fas/FADD-mediated activation of a specific program of inflammatory gene expression in vascular smooth muscle cells. Nat Med. 2000;6:790–796. [PubMed]
3. Lauber K, Bohn E, Krober SM, Xiao YJ, Blumenthal SG, et al. Apoptotic cells induce migration of phagocytes via caspase-3-mediated release of a lipid attraction signal. Cell. 2003;113:717–730. [PubMed]
4. Bournazou I, Pound JD, Duffin R, Bournazos S, Melville LA, et al. Apoptotic human cells inhibit migration of granulocytes via release of lactoferrin. J Clin Invest. 2009;119:20–32. [PMC free article] [PubMed]
5. Ravichandran KS. Find-me and eat-me signals in apoptotic cell clearance: progress and conundrums. The Journal of experimental medicine. 2010;207:1807–1817. [PMC free article] [PubMed]
6. Ravichandran KS. Beginnings of a good apoptotic meal: the find-me and eat-me signaling pathways. Immunity. 2011;35:445–455. [PMC free article] [PubMed]
7. Chekeni FB, Ravichandran KS. The role of nucleotides in apoptotic cell clearance: implications for disease pathogenesis. Journal of molecular medicine. 2011;89:13–22. [PMC free article] [PubMed]
8. Hamet P, deBlois D. Endothelial and myocyte apoptosis–role of angiotensin II. Can J Cardiol. 2001;17(Suppl A):26A–28A. [PubMed]
9. Baumgartner-Parzer SM, Wagner L, Pettermann M, Grillari J, Gessl A, et al. High-glucose–triggered apoptosis in cultured endothelial cells. Diabetes. 1995;44:1323–1327. [PubMed]
10. Sata M, Walsh K. Oxidized LDL activates fas-mediated endothelial cell apoptosis. J Clin Invest. 1998;102:1682–1689. [PMC free article] [PubMed]
11. Cailhier JF, Laplante P, Hebert MJ. Endothelial apoptosis and chronic transplant vasculopathy: recent results, novel mechanisms. Am J Transplant. 2006;6:247–253. [PubMed]
12. Raymond M, Désormeaux A, Laplante P, Vigneault N, Filep J, et al. Apoptosis of endothelial cells triggers a caspase-dependent anti-apoptotic paracrine loop active on vascular smooth muscle cells. FASEB J. 2004;18:705–707. doi: 710.1096/fj.1003-0573fje. [PubMed]
13. Laplante P, Raymond MA, Gagnon G, Vigneault N, Sasseville AMJ, et al. Novel fibrogenic pathways are activated in response to endothelial apoptosis: implications in the pathophysiology of systemic sclerosis. J Immunol. 2005;174:5740–5749. [PubMed]
14. Weigert A, Johann AM, von Knethen A, Schmidt H, Geisslinger G, et al. Apoptotic cells promote macrophage survival by releasing the anti-apoptotic mediator sphingosine-1-phosphate. Blood. 2006;108(5):1635–1642. [PubMed]
15. Sirois I, Raymond MA, Brassard N, Cailhier JF, Fedjaev M, et al. Caspase-3-dependent export of TCTP: a novel pathway for antiapoptotic intercellular communication. Cell Death Differ. 2011;18:549–562. [PMC free article] [PubMed]
16. Chen W, Frank ME, Jin W, Wahl SM. TGF-beta released by apoptotic T cells contributes to an immunosuppressive milieu. Immunity. 2001;14:715–725. [PubMed]
17. Lepage S, Cailhier JF. Chronic transplant vasculopathy microenvironment present in the renal allograft reprograms macrophage phenotype. Transplant Proc. 2009;41:3311–3313. [PubMed]
18. Rovere P, Vallinoto C, Bondanza A, Crosti MC, Rescigno M, et al. Bystander apoptosis triggers dendritic cell maturation and antigen-presenting function. J Immunol. 1998;161:4467–4471. [PubMed]
19. Sean Eardley K, Cockwell P. Macrophages and progressive tubulointerstitial disease. Kidney Int. 2005;68:437–455. [PubMed]
20. Kluth DC, Erwig LP, Rees AJ. Multiple facets of macrophages in renal injury. Kidney Int. 2004;66:542–557. [PubMed]
21. Cailhier JF, Sawatzky DA, Kipari T, Houlberg K, Walbaum D, et al. Resident pleural macrophages are key orchestrators of neutrophil recruitment in pleural inflammation. Am J Respir Crit Care Med. 2006;173:540–547. [PMC free article] [PubMed]
22. Cailhier JF, Partolina M, Vuthoori S, Wu S, Ko K, et al. Conditional macrophage ablation demonstrates that resident macrophages initiate acute peritoneal inflammation. J Immunol. 2005;174:2336–2342. [PubMed]
23. Lin SL, Castano AP, Nowlin BT, Lupher ML, Jr, Duffield JS. Bone marrow Ly6Chigh monocytes are selectively recruited to injured kidney and differentiate into functionally distinct populations. J Immunol. 2009;183:6733–6743. [PubMed]
24. Duffield JS, Forbes SJ, Constandinou CM, Clay S, Partolina M, et al. Selective depletion of macrophages reveals distinct, opposing roles during liver injury and repair. J Clin Invest. 2005;115:56–65. [PMC free article] [PubMed]
25. Martinet W, Verheye S, De Meyer GR. Selective depletion of macrophages in atherosclerotic plaques via macrophage-specific initiation of cell death. Trends in cardiovascular medicine. 2007;17:69–75. [PubMed]
26. De Meyer I, Martinet W, De Meyer GR. Therapeutic strategies to deplete macrophages in atherosclerotic plaques. British journal of clinical pharmacology. 2012 doi: 10.1111/j.1365-2125.2012.04211.x. [PMC free article] [PubMed]
27. Libby P. Inflammation in atherosclerosis. Nature. 2002;420:868–874. [PubMed]
28. Kitchens WH, Chase CM, Uehara S, Cornell LD, Colvin RB, et al. Macrophage depletion suppresses cardiac allograft vasculopathy in mice. Am J Transplant. 2007;7:2675–2682. [PubMed]
29. Stout RD, Jiang C, Matta B, Tietzel I, Watkins SK, et al. Macrophages sequentially change their functional phenotype in response to changes in microenvironmental influences. J Immunol. 2005;175:342–349. [PubMed]
30. Voll RE, Herrmann M, Roth EA, Stach C, Kalden JR, et al. Immunosuppressive effects of apoptotic cells [letter]. Nature. 1997;390:350–351. [PubMed]
31. Fadok VA, Bratton DL, Konowal A, Freed PW, Westcott JY, et al. Macrophages that have ingested apoptotic cells in vitro inhibit proinflammatory cytokine production through autocrine/paracrine mechanisms involving TGF-beta, PGE2, and PAF. J Clin Invest. 1998;101:890–898. [PMC free article] [PubMed]
32. Golpon HA, Fadok VA, Taraseviciene-Stewart L, Scerbavicius R, Sauer C, et al. Life after corpse engulfment: phagocytosis of apoptotic cells leads to VEGF secretion and cell growth. Faseb J. 2004;18:1716–1718. [PubMed]
33. Mosser DM, Edwards JP. Exploring the full spectrum of macrophage activation. Nat Rev Immunol. 2008;8:958–969. [PMC free article] [PubMed]
34. Hanayama R, Tanaka M, Miwa K, Shinohara A, Iwamatsu A, et al. Identification of a factor that links apoptotic cells to phagocytes. Nature. 2002;417:182–187. [PubMed]
35. Jinushi M, Nakazaki Y, Dougan M, Carrasco DR, Mihm M, et al. MFG-E8-mediated uptake of apoptotic cells by APCs links the pro- and antiinflammatory activities of GM-CSF. J Clin Invest. 2007;117:1902–1913. [PMC free article] [PubMed]
36. Aziz MM, Ishihara S, Mishima Y, Oshima N, Moriyama I, et al. MFG-E8 attenuates intestinal inflammation in murine experimental colitis by modulating osteopontin-dependent alphavbeta3 integrin signaling. J Immunol. 2009;182:7222–7232. [PubMed]
37. Cailhier JF, Sirois I, Laplante P, Lepage S, Raymond MA, et al. Caspase-3 activation triggers extra-cellular cathepsin L release and endorepellin proteolysis. J Biol Chem. 2008;283(40):27220–27229. [PubMed]
38. Laplante P, Sirois I, Raymond MA, Kokta V, Beliveau A, et al. Caspase-3-mediated secretion of connective tissue growth factor by apoptotic endothelial cells promotes fibrosis. Cell death and differentiation. 2010;17:291–303. [PubMed]
39. Cornell LD, Smith RN, Colvin RB. Kidney transplantation: mechanisms of rejection and acceptance. Annual review of pathology. 2008;3:189–220. [PubMed]
40. Truman LA, Ford CA, Pasikowska M, Pound JD, Wilkinson SJ, et al. CX3CL1/fractalkine is released from apoptotic lymphocytes to stimulate macrophage chemotaxis. Blood. 2008;112(13):5026–5036. [PubMed]
41. Elliott MR, Chekeni FB, Trampont PC, Lazarowski ER, Kadl A, et al. Nucleotides released by apoptotic cells act as a find-me signal to promote phagocytic clearance. Nature. 2009;461:282–286. [PMC free article] [PubMed]
42. Scannell M, Flanagan MB, deStefani A, Wynne KJ, Cagney G, et al. Annexin-1 and peptide derivatives are released by apoptotic cells and stimulate phagocytosis of apoptotic neutrophils by macrophages. J Immunol. 2007;178:4595–4605. [PubMed]
43. Thery C, Regnault A, Garin J, Wolfers J, Zitvogel L, et al. Molecular characterization of dendritic cell-derived exosomes. Selective accumulation of the heat shock protein hsc73. J Cell Biol. 1999;147:599–610. [PMC free article] [PubMed]
44. Cui T, Miksa M, Wu R, Komura H, Zhou M, et al. Milk fat globule epidermal growth factor 8 attenuates acute lung injury in mice after intestinal ischemia and reperfusion. Am J Respir Crit Care Med. 2010;181:238–246. [PMC free article] [PubMed]
45. Atabai K, Jame S, Azhar N, Kuo A, Lam M, et al. Mfge8 diminishes the severity of tissue fibrosis in mice by binding and targeting collagen for uptake by macrophages. J Clin Invest. 2009;119:3713–3722. [PMC free article] [PubMed]
46. Aziz M, Jacob A, Matsuda A, Wu R, Zhou M, et al. Pre-treatment of recombinant mouse MFG-E8 downregulates LPS-induced TNF-alpha production in macrophages via STAT3-mediated SOCS3 activation. PLoS One. 2011;6:e27685. [PMC free article] [PubMed]
47. Jinushi M, Chiba S, Yoshiyama H, Masutomi K, Kinoshita I, et al. Tumor-associated macrophages regulate tumorigenicity and anticancer drug responses of cancer stem/initiating cells. Proc Natl Acad Sci USA. 2011;108(30):12425–12430. [PMC free article] [PubMed]

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