Mediators of Inflammation

Mediators of Inflammation / 2013 / Article

Research Article | Open Access

Volume 2013 |Article ID 950273 | 8 pages |

Clearance of Apoptotic Cells by Macrophages Induces Regulatory Phenotype and Involves Stimulation of CD36 and Platelet-Activating Factor Receptor

Academic Editor: Hidde Bult
Received10 Jul 2013
Revised14 Sep 2013
Accepted08 Oct 2013
Published20 Nov 2013


Phagocytosis of apoptotic cells (efferocytosis) induces macrophage differentiation towards a regulatory phenotype (IL-10high/IL-12p40low). CD36 is involved in the recognition of apoptotic cells (AC), and we have shown that the platelet-activating factor receptor (PAFR) is also involved. Here, we investigated the contribution of PAFR and CD36 to efferocytosis and to the establishment of a regulatory macrophage phenotype. Mice bone marrow-derived macrophages were cocultured with apoptotic thymocytes, and the phagocytic index was determined. Blockage of PAFR with antagonists or CD36 with specific antibodies inhibited the phagocytosis of AC (~70–80%). Using immunoprecipitation and confocal microscopy, we showed that efferocytosis increased the CD36 and PAFR colocalisation in the macrophage plasma membrane; PAFR and CD36 coimmunoprecipitated with flotillin-1, a constitutive lipid raft protein, and disruption of these membrane microdomains by methyl-β-cyclodextrin reduced AC phagocytosis. Efferocytosis induced a pattern of cytokine production, IL-10high/IL-12p40low, that is, characteristic of a regulatory phenotype. LPS potentiated the efferocytosis-induced production of IL-10, and this was prevented by blocking PAFR or CD36. It can be concluded that phagocytosis of apoptotic cells engages CD36 and PAFR, possibly in lipid rafts, and this is required for optimal efferocytosis and the establishment of the macrophage regulatory phenotype.

1. Introduction

Clearance of apoptotic cells (AC) by macrophages, also called efferocytosis, plays a central role in tissue homeostasis, and the impaired clearance of altered cells has been associated with the development of autoimmune and chronic inflammatory diseases [1]. Macrophages can acquire distinct phenotypes depending on the stimulus. M1 or classically activated macrophages are induced by the recognition of PAMPs (pathogen associated molecular patterns) and by proinflammatory cytokines. These cells exhibit high microbicidal activity and induce inflammation. In contrast, M2 macrophages produce anti-inflammatory and tissue remodelling cytokines and can be divided into subtypes according to the stimulus; the alternatively activated macrophages are induced by Th2 cytokines, and the regulatory macrophages are induced by anti-inflammatory cytokines, immune complexes, apoptotic cells, and oxidised lipids, among other stimuli [2, 3].

The first evidence that efferocytosis induces a suppressor phenotype came from the studies of Fadok et al. [4]. The authors showed that the addition of apoptotic cells to macrophages inhibited the expression of proinflammatory cytokines induced by LPS. Later on, it was reported that the clearance of apoptotic neutrophils induced an IL-10high/IL-12low regulatory phenotype in macrophages [5].

There is evidence that platelet-activating factor (PAF) or PAF-like moieties present in the tumour microenvironment promote tumour growth by suppressing macrophage functions [6]. The addition of apoptotic cells to a subtumorigenic dose of melanoma cells promoted tumour growth, and this phenomenon was significantly reduced when an antagonist of the PAF receptor (PAFR) was injected into the tumour site [7]. Also, phagocytosis of AC has been shown to be decreased by the pretreatment of macrophages with antagonists of PAFR [8]. Moreover, PAFR was shown to be involved in the systemic immunosuppression induced by environmental stressor agents, such as UV radiation and cigarette smoke [9, 10].

The membrane of AC exhibits oxidised phospholipids, which are not present in viable cells. Macrophages recognise these modified lipids through a group of receptors known as “scavenger receptors” [11]. It is well established that CD36 is one of the main “scavenger” receptors involved in the recognition of modified lipids, including oxidised LDL (oxLDL) [11, 12]. We showed cross-desensitisation between oxLDL and PAF [8] and that engagement of both CD36 and PAFR is required for the optimal uptake of oxLDL [13, 14]. In the present study, we investigated the contribution of each receptor for phagocytosis of AC and for the induction of a regulatory phenotype (IL-10high/IL-12p40low) in murine bone marrow-derived macrophages.

2. Materials and Methods

2.1. Cell Culture

Male, 6–8-week-old C57BL/6 mice were obtained from our own animal facilities and were housed in a 12 h light/dark cycle room with water and food ad libitum. Animal care and research protocols were in accordance with the principles and guidelines adopted by the Brazilian College of Animal Experimentation (COBEA) and approved by the Biomedical Sciences Institute/USP-Ethical Committee for Animal Research (CEEA). Bone marrow-derived macrophages (BMDM) were obtained as previously described by Davies and Gordon [15], with minor modifications. In brief, femurs were flushed with DMEM (Dulbecco’s modified eagle medium containing 2 mM l-glutamine, 100 U/mL penicillin G, and 100 mg/mL streptomycin, all from Gibco, Long Island, NY, USA), using a 26-G x 1/2′′ needle. Cells were grown in DMEM containing 20% LCM (L-929 cell conditioned medium) and 15% of heat-inactivated foetal calf serum (FCS), incubated at 37°C in 5% CO2. On day 3, new fresh DMEM with LCM was added. A monolayer of macrophages was scraped on day 6 (96% of the cells were positive for CD11b and F4/80). Macrophages were cultured in DMEM with 5% FCS for one day before the experiments.

2.2. Induction of Apoptosis

Apoptosis of thymocytes was performed as described previously [16]. Briefly, thymuses from young (5-6 weeks old) male C57BL/6 mice were harvested and macerated. A suspension of thymocytes at a concentration of 1 × 106 cells/mL was incubated with 1 μM of dexamethasone (Sigma-Aldrich, St. Louis, MO, USA) for 6 h in DMEM with 10% FCS. Before addition to the macrophages, apoptotic thymocytes were washed three times for the removal of dexamethasone.

2.3. Cell Treatment

The blockage of PAFR was performed using the chemically unrelated antagonists WEB (WEB2086 from Tocris, Bristol, UK) and CV (CV3988 from Enzo Lifesciences, Farmingdale, NY, USA), which were added to macrophages 30 min prior to the addition of apoptotic cells. The concentration of WEB (50 μM) and CV (10 μM) used here was based on previous works by our group [8, 17]. CD36 was blocked by a specific anti-CD36 blocking antibody (monoclonal IgA anti-CD36, clone CRF D-2712, BD Biosciences, Franklin Lakes, NJ, USA) at 1 μg/mL, added 30 min before the addition of AC. The disruption of lipid rafts was performed by depleting cholesterol from membranes with 1 mM methyl-β-cyclodextrin (βCD) or with the inactive analogue α-cyclodextrin (αCD) (all from Sigma-Aldrich, St. Louis, MO, USA) 10 min prior to AC.

2.4. Phagocytosis of Apoptotic Cells

To determine the phagocytic index, macrophages were allowed to adhere to glass coverslips inside 24-well culture microplates. On the next day, nonadherent cells were removed, macrophages were treated with drugs or blocking antibody (WEB, CV, βCD, αCD, vehicle or CD36 Ab, and control Ab), and 10 AC per macrophage were added for phagocytosis for 90 min. The noningested cells were removed and coverslips were stained with haematoxylin and eosin. Results are expressed as a phagocytic index, which was derived by multiplying the percentage of macrophages containing at least one ingested AC by the number of targets ingested by the macrophages.

2.5. Coimmunoprecipitation and Immunoblotting

Macrophages were treated with PAF (10−7 M) (Cayman Chemical, Ann Arbor, Michigan, USA) or apoptotic cells (10 per macrophage) for 20 min. After washing and resting, activated cells were lysed without agitation on ice for 30 min using HEPES buffer containing 1 mM CaCl2, 1 mM MgCl2, 1% Triton X-100, protease inhibitor cocktail (Sigma-Aldrich, St. Louis, MO, USA), and phosphatase inhibitors (NaF and Na3VO4 (Calbiochem-Merck Chemicals, Nottingham, UK). Lysates were incubated overnight with the primary antibody of interest (rabbit anti-PAFR or mouse IgA anti-CD36) at 4°C with gentle agitation. Protein A-Sepharose (GE Healthcare, NJ, USA) and protein G-Sepharose (Amersham-Pharmacia Biotech, Uppsala, Sweden) were added to samples containing anti-PAFR or anti-CD36, respectively, and incubated for 3 h at 4°C with gentle agitation. Immune complexes bound to beads were washed three times with HEPES buffer containing protease and phosphatase inhibitors, without Triton X-100, and boiled in SDS sample buffer for 5 minutes. Proteins were separated by 10% SDS-PAGE, transferred to a Hybond nitrocellulose membrane (GE Healthcare, NJ, USA), and incubated with rabbit-anti-PAFR (Cayman Chemical, Ann Arbor, Michigan, USA), mouse IgA-anti-CD36 (BD Biosciences, Franklin Lakes, NJ, USA) or mouse anti-flotillin-1 (BD Biosciences, Franklin Lakes, NJ, USA). As secondary antibodies, we used anti-rabbit IgG-HPR (1 : 2000), anti-mouse-HRP (1 : 1000) (Cell Signaling Technology, Beverly, MA, USA), biotin-anti-IgA (1 : 500) (BD Biosciences, Franklin Lakes, NJ, USA) with streptavidin-HRP (1 : 200) (Life Technologies, Carlsbad, CA, USA) and visualised using SuperSignal West Pico Chemiluminescent Substrate (Thermo Scientific, Rockford, IL, USA). The resulting autoradiograms were analysed with the AlphaEaseFC software V3.2 beta (Alpha Innotech, San Leandro, CA, USA).

2.6. Confocal Microscopy

Macrophages were plated on glass cover slips and treated with apoptotic cells (10 per macrophage) for 20 minutes. After gentle washing with PBS, cells were fixed with 3% paraformaldehyde. Cells were blocked with 1% BSA in PBS before incubation with primary antibodies including anti-PAFR (1 : 100) (Cayman Chemical, Ann Arbor, Michigan, USA) and IgA anti-CD36 (1 : 100) (BD Biosciences, Franklin Lakes, NJ, USA). Alexa Fluor 647 goat anti-rabbit IgG (1 : 100) (Invitrogen-Life Technologies, Carlsbad, CA, USA) and biotin-anti-mouse IgA (1 : 200) with streptavidin-PE (1 : 200) (BD Biosciences, Franklin Lakes, NJ, USA) were used as secondary antibodies. Cells stained with secondary antibody and control antibody were used to control for the background from each fluorophore. Slides were mounted in Prolong Gold antifade reagent with DAPI (4,6-diamidino-2-phenylindole) (Invitrogen-Life Technologies, Carlsbad, CA, USA). Cells were imaged on a Zeiss LSM 510 confocal microscope using the 100x oil objective. Confocal images were taken with identical settings to allow the comparison of staining. Single confocal sections of the cells were captured in multitrack. Each set of frames from a given treatment condition depicts a representative from at least 20 analysed cells in three independent experiments. Colocalisation was quantified by analysing at least 10 images and determining Pearson’s coefficient using JACoP (Just Another Colocalisation Plugin), and the software ImageJ 1.46r (NIH, USA), which is available at [18]. Basically, a linear equation is calculated to describe the relationship between the intensities in two images (separate colours). The slope of this linear approximation provides the rate of association of two fluorochromes, and Pearson’s coefficient estimates the goodness of this approximation [19].

2.7. Cytokine Measurement

Macrophages were treated with drugs/blocking antibody (WEB, CV, βCD, αCD, or CD36 Ab, 30 min before addition of AC (10 per macrophage)). After 24 h of phagocytosis, one group was stimulated with LPS (10 ng/mL) for 24 h. The supernatants were centrifuged for the removal of noningested cells, and levels of IL-10 and IL-12p40 were measured using a BD OptEIA kit (BD Biosciences, San Diego, CA, USA) according to the manufacturer’s specifications.

2.8. Statistical Analysis

Data are presented as mean ± standard error mean (SEM). Analysis of variance (ANOVA) and the Student-Newman-Keuls posttest were used to evaluate the statistical significance of the differences between three or more groups. A two-tailed unpaired Student’s -test was used when differences between two groups were analysed. Significance was assumed when .

3. Results

3.1. Efferocytosis Is Dependent on the Engagement of PAFR and CD36

To investigate whether the engagement of both PAFR and CD36 is required for macrophages to phagocytose AC, murine macrophages were pretreated with two chemically unrelated antagonists, WEB2086 and CV3988, and CD36 was blocked by a specific antibody. Figure 1 shows that PAFR antagonists decreased the phagocytosis of AC (WEB 71% and CV 79%). Blockage of CD36 also reduced the phagocytosis of AC (70%). The simultaneous blockage of CD36 and PAFR was even more effective at inhibiting the phagocytosis of AC (90 and 93% for association of CD36 with WEB2086 and CV3988, resp.). These results suggest that both receptors are involved in the phagocytosis of AC by macrophages.

We then investigated the possibility of physical interaction between these receptors by evaluating whether phagocytosis of apoptotic cells induces the coimmunoprecipitation and colocalisation of CD36 with PAFR. We found that the addition of AC to macrophages induced the immunoprecipitation of PAFR and CD36, detected within 20 min (Figure 2(a)). A basal coprecipitation of PAFR and CD36 was also observed in resting (control) macrophages, which was not increased after the stimulation of PAFR by the agonist PAF alone. This was reinforced by colocalisation analysis performed by confocal microscopy. Macrophages incubated with AC were labelled with antibodies to CD36 (red) and PAFR (green). We found in AC-treated macrophages, in contrast to the control and PAF-treated macrophages, that there was a redistribution of PAFR and CD36, increasing their colocalisation (2-fold), as shown by the enhanced yellow spots on the macrophage plasma membrane, visualised in Figure 2(b) and quantified in Figure 2(c). As the samples were not permeabilised, the CD36 and PAFR fluorescence observed reflects the presence of these receptors in the cell membrane. Based on this, we can conclude that the overlap of CD36 and PAFR observed in Figure 2(b) occurs on the cell membrane. These data strongly suggest that AC induces a spatial redistribution of PAFR and CD36 in the plasma membrane, resulting in increased immunoprecipitation and colocalisation of these receptors.

Lipid rafts are specialised microdomains in the plasma membrane that allow interactions between receptors. To investigate whether intact lipid rafts are required for the phagocytosis of AC, the phagocytic index was assessed after the treatment of macrophages with methyl-β-cyclodextrin (βCD), which depletes cholesterol from the membrane, causing a disruption of lipid rafts. We found that the ingestion of apoptotic cells was reduced after macrophages were treated with βCD (Figure 3(a)), unlike macrophages that were treated with alpha-cyclodextrin (αCD; chemically-related to βCD, used as a control with no effect in lipid rafts). Furthermore, immunoprecipitation assays were performed for the detection of flotillin-1, which is a protein that is typically found in lipid rafts [20]. Figure 3(b) shows that, in macrophages that have ingested apoptotic cells, the amount of flotillin-1 was significantly increased in the samples immunoprecipitated with antibodies to CD36. Likewise, in the samples immunoprecipitated with antibodies to PAFR, the amount of flotillin-1 was also increased. Together, these results show that when apoptotic cells interact with macrophages, PAFR and CD36 are recruited to the lipid rafts and that the integrity of these membrane domains is required for the optimal ingestion of apoptotic cells.

3.2. PAFR and CD36 Contribute to the Induction of a Regulatory Phenotype in Macrophages during Efferocytosis

We next evaluated the phenotype of macrophages that have ingested AC by measuring the production of IL-12p40 and IL-10. Figure 4(a) shows that these macrophages produced IL-10 and small amounts of IL-12p40. In order to potentiate the production of these cytokines, LPS was added to macrophages 24 h after efferocytosis. In these conditions, the production of IL-10, increased whereas IL-12p40 was not affected, resulting in an IL-10high/IL-12low phenotype, which is characteristic of regulatory macrophages. We then evaluated the effect of PAFR antagonists, anti-CD36 antibodies, or the combination of both on cytokine production. Figure 4(b) shows that the blockage of PAFR or CD36 inhibited efferocytosis-induced IL-10 production without affecting IL-12p40. In the case of treatment with the PAFR antagonist CV3988, the IL-10/IL-12p40 ratio changed from 1.4 in the nontreated to 0.6 in the antagonist-treated macrophages. Blocking CD36 or both PAFR and CD36 had a similar effect, redirecting macrophages towards a more activated profile by favouring higher amounts of IL-12p40 relative to IL-10. These results show that, during efferocytosis, macrophages acquire an IL-10high/IL-12p40low cytokine production profile and that both PAFR and CD36 are involved in the establishment of a regulatory phenotype in macrophages that have ingested AC.

4. Discussion

Here, we showed that engagement of both PAFR and CD36 is required for the phagocytosis of apoptotic cells and for the induction of the IL-10high/IL-12p40low profile (regulatory) that follows efferocytosis. In addition, we showed that efferocytosis increased the colocalisation of these receptors and immunoprecipitation with the membrane lipid raft marker protein flotillin-1; also we demonstrated that lipid raft integrity is required for the optimal ingestion of AC. To our knowledge, this is the first study to suggest that PAFR and CD36 co-localise and are recruited to lipid raft microdomains during efferocytosis and that the engagement of both receptors is required for AC ingestion and the induction of a regulatory phenotype of macrophages.

Both PAFR and CD36 recognise modified/oxidised lipids and share common ligands, such as oxLDL and moieties present in the membrane of apoptotic cells, as shown here. Recently, we showed that co-stimulation of PAFR and CD36 is required for the uptake of oxLDL and for the induction of cytokine genes by oxLDL [13, 14]. Here, we showed that recognition and phagocytosis of apoptotic cells were also dependent on PAFR and CD36. This was shown by using two chemically unrelated PAFR antagonists and by blocking CD36 with a specific antibody. Interestingly, the simultaneous blockage of both receptors had an additive effect in efferocytosis inhibition. These results suggest that moieties present in the AC membrane engage both receptors, and that this is required for the ingestion of AC. Furthermore, we were able to demonstrate by immunoprecipitation and confocal microscopy that efferocytosis caused an increase in CD36 and PAFR colocalisation. Since the samples were not permeabilised, we can conclude that the overlap of CD36 and PAFR occurs in the cell membrane. However, the possibility of interactions between receptors in the phagosome membrane after apoptotic cell ingestion or even on cytoplasmic compartments cannot be ruled out.

The dynamics and trafficking of membrane receptors involve the formation of lipid rafts (LR), which are cholesterol- and sphingomyelin-rich membrane microdomains that function as platforms to promote the association of signalling molecules and the compartmentalisation of cellular processes [21]. It has been shown that CD36 is recruited to lipid rafts in a ligand-dependent manner [22, 23], and that PAFR has a binding motif for a constitutive protein of lipid rafts (caveolin-1) in its sequence [24]. Here, we showed that, during efferocytosis, PAFR and CD36 co-immunoprecipitated with flotillin-1, which is a protein that is typically found in lipid rafts and is used as a protein marker to detect these microdomains. When LR were disrupted by cholesterol with βCD, efferocytosis was reduced, suggesting a requirement of LR integrity for ingestion of AC. Structures like LR permit receptors with a nontransducing short intracytoplasmic portion, like CD36, to come into close proximity with other receptors promoting interactions that allow signalling. These results show that efferocytosis increases the colocalisation of PAFR and CD36 in the macrophage plasma membrane, and that this colocalisation probably happens in the same LR. Although there must be other receptors docked in these LR, these data strongly suggest that PAFR and CD36 interact to achieve optimal efferocytosis.

Regulatory macrophages can be generated by several stimuli such as Fcγ and toll-like receptor ligands, glucocorticoids, prostaglandins, and apoptotic cells [2, 3, 25]. The major feature of regulatory macrophages is their anti-inflammatory ability due to the production of high levels of IL-10, a potent cytokine with inhibitory effect on immune response, and low levels of IL-12, which has an effect that is opposite to that of IL-10. The balance of IL-10 and IL-12 production has been previously employed to establish the polarisation of macrophage phenotype [5, 26, 27]. We showed here that phagocytosis of apoptotic cells induces more IL-10 than IL-12p40. When macrophages that have ingested apoptotic cells were stimulated with LPS, they produced significantly higher levels of IL-10 than those that had not been exposed to apoptotic cells. This was not observed with IL-12, where the increased levels induced by LPS were not further increased by the phagocytosis of apoptotic cells. Phagocytosis of apoptotic cells by human macrophages even decreased the production of IL-12p70 induced by LPS and IFN-γ, as described by Kim et al. [28]. This difference may be explained by the following: they used human macrophages and we used bone marrow-derived murine macrophages; they activated the cells with LPS plus IFN-γ and we used only LPS; and they measured the subunit p70 of IL-12, whereas in our case we used p40. In our study, the ratio between IL-10 and IL-12 was increased by efferocytosis, leading to the IL-10high/IL-12p40low phenotype, which is characteristic of regulatory macrophages. Moreover, this enhancement of the IL-10/IL-12 ratio was dependent on both PAFR and CD36 engagement, suggesting that both receptors are involved in macrophage polarisation towards a regulatory phenotype.

In a previous study, we observed that the injection of a subtumorigenic dose of melanoma cells together with apoptotic cells promoted tumour growth and that PAFR antagonists prevented this effect [7]. This suggests that PAFR antagonists, by inhibiting AC recognition, can prevent macrophages from acquiring the regulatory phenotype; and thus the blocking of PAFR during tumour growth could be of therapeutic interest. Another consequence of blocking PAFR is the potential reduction of foam cell formation due to the inhibition of oxLDL uptake, which would be theoretically desirable in atherosclerosis [13, 14]. On the other hand, we showed here that blocking PAFR and/or CD36 reduces the clearance of apoptotic cells, which is an essential mechanism for maintaining homeostasis. The defective clearance of apoptotic cells was associated with some autoimmune and chronic diseases such as systemic lupus erythematosus, type 1 diabetes, chronic obstructive pulmonary disease, and cardiovascular disease [1]. Clearly, the use of agents that block these receptors should be considered with great care. Moreover, some authors propose regulatory macrophages to be used in protocols for immunomodulation to treat inflammatory and autoimmune diseases [29, 30]. In this case, pretreatment of macrophages with ligands of PAFR and/or CD36 might be useful and may increase their drift towards the regulatory phenotype. The present study added to the knowledge of the mechanisms involved in efferocytosis. It would be desirable to further unravel these mechanisms, with the aim of identifying strategies to treat diseases caused by defective efferocytosis and treatments based on immunomodulatory macrophages.

5. Conclusion

It can be concluded that the phagocytosis of apoptotic cells engages CD36 and PAFR, possibly in lipid rafts, and this is required for optimal efferocytosis and the establishment of the macrophage regulatory phenotype (IL-10high/IL-12p40low).

Conflict of Interests

The authors have no financial conflict of interests.


This study was funded by Fundação de Amparo à Pesquisa do Estado de São Paulo (FAPESP) (Grants 2006/03982-5 and 2009/03368-3) and Conselho Nacional de Desenvolvimento Científico e Tecnológico (CNPq).


  1. D. Korns, S. C. Frasch, R. Fernandez-Boyanapalli, P. M. Henson, and D. L. Bratton, “Modulation of macrophage efferocytosis in inflammation,” Frontiers in Immunology, vol. 2, article 57, 2011. View at: Publisher Site | Google Scholar
  2. D. M. Mosser and J. P. Edwards, “Exploring the full spectrum of macrophage activation,” Nature Reviews Immunology, vol. 8, no. 12, pp. 958–969, 2008. View at: Publisher Site | Google Scholar
  3. J. P. Edwards, X. Zhang, K. A. Frauwirth, and D. M. Mosser, “Biochemical and functional characterization of three activated macrophage populations,” Journal of Leukocyte Biology, vol. 80, no. 6, pp. 1298–1307, 2006. View at: Publisher Site | Google Scholar
  4. V. A. Fadok, D. L. Bratton, A. Konowal, P. W. Freed, J. Y. Westcott, and P. M. Henson, “Macrophages that have ingested apoptotic cells in vitro inhibit proinflammatory cytokine production through autocrine/paracrine mechanisms involving TGF-β, PGE2, and PAF,” Journal of Clinical Investigation, vol. 101, no. 4, pp. 890–898, 1998. View at: Google Scholar
  5. A. A. Filardy, D. R. Pires, M. P. Nunes et al., “Pro-inflammatory clearance of apoptotic neutrophils induces an IL-12(low)IL-10(high) regulatory phenotype in macrophages,” Journal of Immunology, vol. 185, no. 4, pp. 2044–2050, 2010. View at: Publisher Site | Google Scholar
  6. S. Jancar and R. Chammas, “PAF receptor and tumour growth,” Bioactive Lipids in Cancer. In press. View at: Google Scholar
  7. A. L. Bachi, L. C. Dos Santos, S. Nonogaki, S. Jancar, and M. G. Jasiulionis, “Apoptotic cells contribute to melanoma progression and this effect is partially mediated by the platelet-activating factor receptor,” Mediators of Inflammation, vol. 2012, Article ID 610371, 6 pages, 2012. View at: Publisher Site | Google Scholar
  8. S. I. de Oliveira, P. D. Fernandes, J. G. Amarante Mendes, and S. Jancar, “Phagocytosis of apoptotic and necrotic thymocytes is inhibited by PAF-receptor antagonists and affects LPS-induced COX-2 expression in murine macrophages,” Prostaglandins and Other Lipid Mediators, vol. 80, no. 1-2, pp. 62–73, 2006. View at: Publisher Site | Google Scholar
  9. R. P. Sahu, I. Petrache, M. J. Van Demark et al., “Cigarette smoke exposure inhibits contact hypersensitivity via the generation of platelet-activating factor agonists,” The Journal of Immunology, vol. 190, no. 5, pp. 2447–2454, 2013. View at: Google Scholar
  10. R. P. Sahu, M. J. Turner, S. C. DaSilva et al., “The environmental stressor ultraviolet B radiation inhibits murine antitumor immunity through its ability to generate platelet-activating factor agonists,” Carcinogenesis, vol. 33, no. 7, pp. 1360–1367, 2012. View at: Publisher Site | Google Scholar
  11. Y. I. Miller, S.-H. Choi, P. Wiesner et al., “Oxidation-specific epitopes are danger-associated molecular patterns recognized by pattern recognition receptors of innate immunity,” Circulation Research, vol. 108, no. 2, pp. 235–248, 2011. View at: Publisher Site | Google Scholar
  12. V. V. Kunjathoor, M. Febbraio, E. A. Podrez et al., “Scavenger receptors class A-I/II and CD36 are the principal receptors responsible for the uptake of modified low density lipoprotein leading to lipid loading in macrophages,” Journal of Biological Chemistry, vol. 277, no. 51, pp. 49982–49988, 2002. View at: Publisher Site | Google Scholar
  13. F. J. O. Rios, M. Gidlund, and S. Jancar, “Pivotal role for platelet-activating factor receptor in CD36 expression and oxLDL uptake by human monocytes/macrophages,” Cellular Physiology and Biochemistry, vol. 27, no. 3-4, pp. 363–372, 2011. View at: Publisher Site | Google Scholar
  14. F. J. O. Rios, M. M. Koga, M. Ferracini, and S. Jancar, “Co-stimulation of PAFR and CD36 is required for oxLDL-induced human macrophages activation,” PLoS ONE, vol. 7, no. 5, Article ID e36632, 2012. View at: Publisher Site | Google Scholar
  15. J. Q. Davies and S. Gordon, “Isolation and culture of murine macrophages,” Methods in Molecular Biology, vol. 290, pp. 91–103, 2005. View at: Google Scholar
  16. B. Hu, A. Punturieri, J. Todt, J. Sonstein, T. Polak, and J. L. Curtis, “Recognition and phagocytosis of apoptotic T cells by resident murine tissue macrophages require multiple signal transduction events,” Journal of Leukocyte Biology, vol. 71, no. 5, pp. 881–889, 2002. View at: Google Scholar
  17. S. I. de Oliveira, L. N. S. Andrade, A. C. Onuchic et al., “Platelet-activating factor receptor (PAF-R)-dependent pathways control tumour growth and tumour response to chemotherapy,” BMC Cancer, vol. 10, article 200, 2010. View at: Publisher Site | Google Scholar
  18. C. A. Schneider, W. S. Rasband, and K. W. Eliceiri, “NIH Image to ImageJ: 25 years of image analysis,” Nature Methods, vol. 9, no. 7, pp. 671–675, 2012. View at: Google Scholar
  19. S. Bolte and F. P. Cordelières, “A guided tour into subcellular colocalization analysis in light microscopy,” Journal of Microscopy, vol. 224, no. pt 3, pp. 213–232, 2006. View at: Publisher Site | Google Scholar
  20. A. Auriac, A. Willemetz, and F. Canonne-Hergaux, “Lipid raft-dependent endocytosis: A new route for hepcidin-mediated regulation of ferroportin in macrophages,” Haematologica, vol. 95, no. 8, pp. 1269–1277, 2010. View at: Publisher Site | Google Scholar
  21. D. Lingwood and K. Simons, “Lipid rafts as a membrane-organizing principle,” Science, vol. 327, no. 5961, pp. 46–50, 2010. View at: Publisher Site | Google Scholar
  22. M. Triantafilou, F. G. J. Gamper, P. M. Lepper et al., “Lipopolysaccharides from atherosclerosis-associated bacteria antagonize TLR4, induce formation of TLR2/1/CD36 complexes in lipid rafts and trigger TLR2-induced inflammatory responses in human vascular endothelial cells,” Cellular Microbiology, vol. 9, no. 8, pp. 2030–2039, 2007. View at: Publisher Site | Google Scholar
  23. Y. Zeng, N. Tao, K.-N. Chung, J. E. Heuser, and D. M. Lublin, “Endocytosis of oxidized low density lipoprotein through scavenger receptor CD36 utilizes a lipid raft pathway that does not require caveolin-1,” Journal of Biological Chemistry, vol. 278, no. 46, pp. 45931–45936, 2003. View at: Publisher Site | Google Scholar
  24. C. Poisson, S. Rollin, S. Véronneau et al., “Caveolae facilitate but are not essential for platelet-activating factor-mediated calcium mobilization and extracellular signal-regulated kinase activation,” Journal of Immunology, vol. 183, no. 4, pp. 2747–2757, 2009. View at: Publisher Site | Google Scholar
  25. S. Gordon, “Alternative activation of macrophages,” Nature Reviews Immunology, vol. 3, no. 1, pp. 23–35, 2003. View at: Publisher Site | Google Scholar
  26. S. E. Elcombe, S. Naqvi, M. W. Van Den Bosch et al., “Dectin-1 regulates IL-10 production via a MSK1/2 and CREB dependent pathway and promotes the induction of regulatory macrophage markers,” PLoS ONE, vol. 8, no. 3, Article ID e60086, 2013. View at: Publisher Site | Google Scholar
  27. K. F. MacKenzie, K. Clark, S. Naqvi et al., “PGE(2) induces macrophage IL-10 production and a regulatory-like phenotype via a protein kinase A-SIK-CRTC3 pathway,” The Journal of Immunology, vol. 190, no. 2, pp. 565–577, 2013. View at: Publisher Site | Google Scholar
  28. S. Kim, K. B. Elkon, and X. Ma, “Transcriptional suppression of interleukin-12 gene expression following phagocytosis of apoptotic cells,” Immunity, vol. 21, no. 5, pp. 643–653, 2004. View at: Publisher Site | Google Scholar
  29. J. S. Gerber and D. M. Mosser, “Reversing lipopolysaccharide toxicity by ligating the macrophage Fcγ receptors,” Journal of Immunology, vol. 166, no. 11, pp. 6861–6868, 2001. View at: Google Scholar
  30. B. D. Fleming and D. M. Mosser, “Regulatory macrophages: Setting the threshold for therapy,” European Journal of Immunology, vol. 41, no. 9, pp. 2498–2502, 2011. View at: Publisher Site | Google Scholar

Copyright © 2013 Matheus Ferracini et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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