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Blood. Author manuscript; available in PMC Jun 11, 2013.
Published in final edited form as:
PMCID: PMC3677739
HALMSID: HALMS605106
INSERM Subrepository
p16INK4a deficiency promotes IL-4-induced polarization and inhibits proinflammatory signaling in macrophages
Céline Cudejko,1 Kristiaan Wouters,1 Lucía Fuentes,1 Sarah Anissa Hannou,1 Charlotte Paquet,1 Kadiombo Bantubungi,1 Emmanuel Bouchaert,1 Jonathan Vanhoutte,1 Sébastien Fleury,1 Patrick Remy,2 Anne Tailleux,1 Giulia Chinetti,1 David Dombrowicz,1 Bart Staels,1* and Réjane Paumelle1
1Récepteurs nucléaires, maladies cardiovasculaires et diabète INSERM : U1011, Institut Pasteur de Lille, Université du Droit et de la Santé - Lille II, 1 rue du Prof Calmette 59019 Lille Cedex,FR
2Service de Production des Antigènes Institut Pasteur de Lille, 1 rue du Professeur Calmette 59019 Lille,FR
* Correspondence should be addressed to: Bart Staels ; bart.staels/at/pasteur-lille.fr
The CDKN2A locus, which contains the tumor suppressor gene p16INK4a, is associated with an increased risk of age-related inflammatory diseases, such as cardiovascular disease and type 2 diabetes, in which macrophages play a crucial role. Monocytes can polarize towards classically (CAM[var phi]) or alternatively (AAM[var phi]) activated macrophages. However, the molecular mechanisms underlying the acquisition of these phenotypes are not well defined.
Here, we show that p16INK4a-deficiency (p16−/−) modulates the macrophage phenotype. Transcriptome analysis revealed that p16−/− bone marrow-derived macrophages (BMDM) exhibit a phenotype resembling interleukin (IL)-4-induced macrophage polarization. In line with this observation, p16−/− BMDM displayed a decreased response to classically polarizing IFNγ and LPS and an increased sensitivity to alternative polarization by IL-4. Furthermore, mice transplanted with p16−/− bone marrow displayed higher hepatic AAM[var phi] marker expression levels upon Schistosoma mansoni infection, an in vivo model of AAM[var phi] phenotype-skewing. Surprisingly, p16−/− BMDM did not display increased IL-4-induced STAT6 signaling, but decreased IFNγ-induced STAT1 and LPS-induced IKKα,β phosphorylation. This decrease correlated with decreased JAK2 phosphorylation and with higher levels of inhibitory acetylation of STAT1 and IKKα,β. These findings identify p16INK4a as a modulator of macrophage activation and polarization via the JAK2-STAT1 pathway with possible roles in inflammatory diseases.
Keywords: Animals, Bone Marrow Transplantation, Cyclin-Dependent Kinase Inhibitor p16, deficiency, physiology, Cytokines, biosynthesis, Genes, p16, I-kappa B Kinase, physiology, Inflammation, genetics, Interferon-gamma, pharmacology, Interleukin-4, pharmacology, Janus Kinase 2, physiology, Lipopolysaccharides, pharmacology, Liver, metabolism, pathology, Macrophage Activation, drug effects, Macrophages, drug effects, physiology, Mice, Mice, Inbred C57BL, Phosphorylation, Protein Processing, Post-Translational, Radiation Chimera, STAT1 Transcription Factor, physiology, STAT6 Transcription Factor, physiology, Schistosomiasis, immunology, Signal Transduction
The tumor suppressor p16INK4a is encoded by the CDKN2A locus on the human chromosome 9p21 and on the murine chromosome 4. p16INK4a belongs to the INK4 family of cyclin-dependent kinase (CDK) inhibitors, also including p15INK4b, p18INK4c, and p19INK4d [15]. p16INK4a inhibits cell cycle progression by preventing cyclin D-CDK 4/6 complex formation. As a consequence, pRb hyperphosphorylation and its association with E2F, which induces transcription of S phase genes, are inhibited. p16INK4a inactivation by deletion, point mutation or promoter methylation, occurs frequently in most tumors [6].
Besides its role in cancer as an inhibitor of cell cycle progression, p16INK4a plays a crucial role in senescence and aging [7,8]. Indeed, expression of p16INK4a increases with age in various tissues from several species [9-11]. A genome-wide association study has shown association of the CDKN2A locus with an increased risk of the age-related frailty syndrome [12]. Additionally, increased p16INK4a expression causes the age-dependent decline in proliferation of self-renewing cellular compartments such as haematopoietic stem cells [13], which give rise to immune cells.
Although the role of p16INK4a in mature immune cells has not yet been investigated, a number of studies has shown that the CDKN2A locus is associated with an increased risk for coronary heart disease [14], atherosclerosis [15], and type 2 diabetes (T2D) [16]. In these pathologies, immune cells, such as macrophages, play a crucial role. Besides their pleiotropic immune functions, macrophages also play a role in the development and homeostasis of several tissues, such as adipose tissue [17] and liver [18]. Depending upon the cytokine environment, macrophages differentiate into distinct subclasses with specific characteristics. Classically activated macrophages (CAM[var phi]) differentiate in presence of Th1 cytokines, such as interferon gamma (IFNγ), or in presence of bacterial products such as lipopolysaccharide (LPS). CAM[var phi] trigger pro-inflammatory responses required to kill intracellular pathogens [19]. Alternatively activated macrophages (AAM[var phi]), induced by Th2 cytokines such as interleukin (IL)-4 and IL-13, are associated with Th2-type immune responses as seen in helminth parasite infections [1]. During inflammation, AAM[var phi] play a key role in protecting the organism against tissue damage [2]. However, little is known about the mechanisms underlying the acquisition of the AAM[var phi] phenotype.
In the present study, we investigated whether p16INK4a-deficiency influences macrophage activation in vitro, using bone marrow-derived macrophages (BMDM), and in vivo by infection with the parasite Schistosoma mansoni. BMDM from p16INK4a-deficient (p16−/−) mice exhibit a phenotype resembling IL-4-induced macrophage polarization and an enhanced response to the Th2 cytokine IL-4 compared to BMDM from wild type (p16+/+) mice. By contrast, their response to Th1 stimuli is diminished. Moreover, Schistosoma mansoni infection of mice transplanted with p16−/− bone marrow resulted in an increased hepatic AAM[var phi] signature in vivo. Finally, we show that p16INK4a-deficiency does not influence the IL-4-induced STAT6 pathway. By contrast, the lower response to classical activation stimuli likely occurs through an inhibition of the phosphorylation of both STAT1 and IKKα,β, which correlated with decreased JAK2 phosphorylation and increased acetylation of STAT1 and IKKα,β,
Mice
C57BL/6J p16INK4a-deficient and littermate control mice on a C57Bl6 background (>97%) were kindly provided by P. Krimpenfort. p16−/− mice showed neither abnormalities in biochemical parameters nor spontaneous tumor development at the studied age. Flow cytometry analysis of splenic T- and B-cells or macrophages showed no differences between p16−/− and p16+/+ mice (data not shown). All protocols were conducted with the approval of the Pasteur Institute ethical review board, Lille, France.
Bone marrow chimeras
8 week-old C57BL/6J mice were lethally irradiated (8 Gy) and injected in the tail vein the next day with 10x106 bone marrow cells isolated from p16−/− or p16+/+ donor mice. Mice were supplied with autoclaved acidified water (pH=2) supplemented with neomycin 100 mg/L (Cat.N1142, Sigma-Aldrich), polymyxin B sulphate 60000 U/L (Cat.21850029, Invitrogen) 1 week before and 4 weeks after transplantation. Mice were studied 6 weeks post-transplantation to allow repopulation by the donor bone marrow. To ensure that donor bone marrow replaced the resident blood cell population, DNA was extracted from whole blood with an Illustra blood kit (GE Healthcare). PCR was performed with forward 5′-GCA-GTG-TTG-CAG-TTT-GAA-CCC-3′ and reverse 5′-TGT-GGC-AAC-TGA-TTC-AGT-TTG-3′ primer sets yielding products of different lengths, which were separated on a 1.5% agarose gel and quantified with the Gel Doc XR system (Bio-Rad). Over 95% of host blood cells were from donor origin.
Primary cell isolation and culture
LPS-elicited neutrophils from air pouches were isolated as described [21]. Splenic CD4+ T-cells and CD43 B-cells were isolated from female mice respectively using Dynal (Invitrogen), biotin-conjugated anti-CD43 (Becton Dickinson) and streptavidin conjugated to magnetic beads (Miltenyi Biotech) according to manufacturer’s instructions. Bone marrow-derived dendritic cells were prepared as described [22]. BMDM were obtained from femoral and tibial bone marrow suspensions, plated at 10x106 cells in 10 cm plates and differentiated in BMDM medium (RPMI 1640 containing Hepes 25 mM supplemented with 10% low endotoxin fetal bovine serum, 15% L929-conditioned medium, 2 mM L-glutamine, 1 mM gentamycine). Stimulations and microarray analysis were carried out at day 8. IL-4 (15 ng/mL) and IFNγ (2.5 ng/mL and 10 ng/mL) were obtained from Peprotech. LPS (100 ng/mL) from E. coli serotype 0111B4 was from Sigma-Aldrich. CINK4 (#219492) was obtained from Merck. For indirect co-culture experiments, conditioned medium of alternatively differentiated p16+/+ and p16−/− macrophages was added to cultures of BMDM 24h before LPS (100 ng/mL) stimulation. After 4h, CAM[var phi] were washed and cultured for 24h in fresh medium. The resulting media were assayed for cytokine secretion by ELISA.
Flow cytometry
During in vitro differentiation, asynchronously growing cultures of BMDM were gently scraped every two days with PBS 1X/EDTA 10 mM/2% trypsine, washed with PBS and collected by centrifugation (5 min, 900 rpm). For protein analysis, non-specific staining was avoided by incubating cells with purified rat anti-mouse CD16/CD32 (Cat.553141, BD Pharmingen) for 20 min at 4°C and labeled with anti-mouse F4/80-FITC (Cat.RM2901, Caltag Laboratories) for 30 min at 4°C. Cells were analyzed using a Coulter EPICS XL4-MCL® Flow cytometer (BeckmanCoulter) and Expo32® software (applied cytometry systems). For cell sorting, cells were incubated with anti-mouse F4/80-FITC antibodies (11-4801, eBioscience) and Rat IgG2a K isotype (11-4321, eBioscience) and sorted on an EPICS-ALTRA cell sorter (Beckman Coulter). For FACS-based cell cycle analysis, cells were fixed with 70% ethanol for 1h at −20°C and labeled with 50 μg/mL propidium iodide containing 50 μg/mL RNase A for 30 min at room temperature. The percentage of cell cycle distribution was obtained using the Multicycle® software (Phoenix Flow systems).
Microarray studies
Mouse genome MOE 430 2.0 gene chips (Affymetrix®) were used in triplicate for each condition. Sample preparation, hybridization and scanning were performed according the One-cycle protocol (Affymetrix®). Only genes significantly regulated (p<0.05) were analyzed further with Genomatix Bibliosphere®. Microarray data have been deposited to http://www.ebi.ac.uk/arrayexpress.
RNA extraction and analysis
Total RNA was obtained from BMDM using EXTRACT-ALL®, DNase-I treated, and cDNA was generated using cDNA reverse transcription kit (AB Applied Biosystems). Real-time QPCR detection was conducted on a Stratagene Mx3005P® (Agilent technologies) using Brilliant II SYBR Green reagent® (Agilent Technologies) and specific primers (Table S1). mRNA levels were normalized to 36B4 mRNA and fold induction was calculated using the 2−ΔΔCt method.
Cytokine production measurement
IL-6, TNF, IL-1Rn, IL-4, IL-10 and IFNγ levels in culture supernatants were measured with ELISA kits according to the manufacturer’s instructions (R&D systems). Plasma IgE from infected animals was determined by ELISA using purified rat anti-mouse IgE (Cat.553416, BD Pharmingen) as a capture antibody, and biotin rat anti-mouse IgE as a detection antibody (Cat.553414, BD Pharmingen). Standards were prepared using purified mouse IgE κ isotype control (Cat.557079, BD Pharmingen).
Protein extraction and Western blotting
BMDM lysates were prepared using Cell Lysis Buffer (#9803, Cell Signaling Technology) supplemented with 1 mM PMSF. Lysates were resolved in 16% or 10% SDS-PAGE and analyzed by western-blot. Anti-p16 (sc-1207), -actin (sc-1616) and -p38 (sc-535) antibodies were purchased from Santa Cruz Biotechnology. Anti-phospho-STAT6 and -STAT6 (#9361 and 9362), anti-phospho-STAT1 and -STAT1 (#9171 and 9172), anti-phospho-p38 (#9211), anti-phospho-IKKα,β (#2681), anti-IκBα (#9242) and anti-phospho-JAK2 and -JAK2 (#3771 and 3230) antibodies were purchased from Cell Signaling Technology. Hybridizations were done 1:1000 in 5% BSA, 1X TBS, 0.1% Tween-20 overnight at 4°C. Anti-rabbit IgG Peroxidase conjugate secondary antibody 1:10000 (Cat.A-0545, Sigma-Aldrich) was added for 1h at room temperature. Signals were visualized using the enhanced chemiluminescence Western blot detection kit (Amersham ECL plus Western blotting Detection System; GE Healthcare). Membranes were stripped with Reblot Plus Strong Antibody Stripping Solution® (Cat.2504, Millipore) and re-blotted with the indicated antibodies.
Immunoprecipitation (IP) assay
500 μg of BMDM lysates were prepared using lysis buffer supplemented with trichostatin A 1 μM (Cat.T8552, Sigma-Aldrich). Lysates were mixed with 100 μL of Protein G/Protein A Agarose (Millipore) and rotated for 1h at 4°C. After centrifugation for 2 min at 3000 rpm, anti-acetyl-Lysine antibody 1:100 (ab21623, Abcam) was added. Samples were rotated overnight at 4°C. The Protein G/Protein A Agarose mix (100 μL) was added to the samples and incubated for 1h at 4°C. The beads were washed 3x and the pellets dissolved in 40 μL of Laemmli 2X buffer. Proteins were analyzed by western blotting as previously described.
S. mansoni infection
Chimeric mice were anesthetized and percutaneously infected with 40 S. mansoni cercariae and sacrificed 9 weeks later. The liver was perfused and adult worms were recovered and quantified. A piece of liver was weighed and dissolved in a KOH solution (5%, 37°C during 16h) and eggs were counted. Organs were snap frozen or fixed in paraformaldehyde for further analysis. Resin-embedded livers were cut at 5 μm and Mallory’s Trichrome staining was performed to determine granuloma size and hepatic collagen. Immunostaining was performed using antibodies directed to Moma-2 (sc59332, Santa Cruz), Arginase1 (Arg-I) (ab60176-100), Fizz1 (ab39626-50) and Ym1 (ab93034) from Abcam. May Grunwald Giemsa staining was performed and eosinophils were counted per granuloma area. Granulomas were isolated using an Arcturus Laser capture microdissection system from 14 μm sections of snap frozen liver samples. For ex vivo restimulation, spleens were homogenized, filtered (70 μm) and erythrocytes were lysed. Cells were cultured in RPMI 1640 (Gibco) supplemented with 10% low endotoxin fetal bovine serum and 1 mM gentamycin. 5x105 cells were stimulated with 10 μg/ml soluble egg antigen (SEA) or anti-CD3 (#555274; BD Pharmingen) antibodies during 4 days after which medium was collected for cytokine determination by ELISA.
Statistical analysis
Groups were compared using 2-tailed non-paired t-tests using GraphPad Prism® software. In vitro data are expressed as means ± SD and in vivo data are expressed as means ± SEM.
p16INK4a expression increases during macrophage maturation, but p16INK4a-deficiency does not modulate macrophage cell cycle progression
In order to assess whether and in which mature immune cell types p16INK4a is expressed, p16INK4a mRNA was measured in dendritic cells (DC), bone marrow-derived macrophages (BMDM) and neutrophils, all of myeloid origin, and in B- and T-lymphocytes. p16INK4a was highly expressed in BMDM and DC, while its expression was markedly lower in neutrophils and virtually absent in lymphocytes (Figure 1A). Since the CDKN2A locus has been associated to diseases with inflammatory components in which macrophages play a central role, we focused on the role of p16INK4a in these cells. BMDM displayed a gradual increase in p16INK4a mRNA expression during in vitro differentiation (Figure 1B). Cell sorting analysis showed that p16INK4a mRNA expression increased specifically in F4/80-positive cells (macrophages) (Figure S1). Together, these data show that increased expression occurs in a higher number of macrophages which also express higher p16INK4a levels. In line, p16INK4a protein was expressed in differentiated macrophages (Figure 1C). Absence of p16INK4a (Figure 1C) did not influence macrophage maturation, since it affected neither mRNA (Figure 1D) nor protein (Figure 1E) expression of the macrophage surface marker F4/80 during differentiation. Interestingly, absence of p16INK4a did not affect cell cycle progression at any time point of in vitro macrophage differentiation (Figure 1F). Expression analysis of the INK4 family members p15INK4b, p18INK4c, p19INK4d and p19ARF, another product of the INK4A/ARF locus which inhibits the p53 pathway, as well as the KIP/CIP family members p21WAF1 and p27KIP1 revealed increased expression of p15INK4b in p16INK4a-deficient (p16−/−) BMDM (Fig. S2). Together with the observation that expression of Cyclin D, a direct E2F target gene, is similar in both genotypes (Figure S3), these data suggest that the induction of p15INK4b may compensate for p16INK4a-deficiency in the control of the cell cycle.
Figure 1
Figure 1
p16INK4a is expressed, but does not influence maturation or the cell cycle in macrophages
These data indicate that p16INK4a expression increases during macrophage differentiation and that p16INK4a-deficiency influences neither maturation nor the cell cycle in BMDM.
Macrophage p16INK4a-deficiency leads to a phenotype resembling IL-4-induced macrophage polarization
Microarray analysis of p16−/− BMDM revealed that the expression of a large number of inflammatory genes was significantly lower compared to wild type (p16+/+) BMDM under basal conditions (Figure 2A). Several of these genes are typically associated with a CAM[var phi] phenotype [2327]. By contrast, a number of AAM[var phi]-associated genes, linked to IL-4-induced STAT6 activation [2327], were significantly higher expressed in p16−/− BMDM (Figure 2B). However, the AAM[var phi] markers Ym1/2 and Fizz1 were not spontaneously induced by p16INK4a-deficiency. The differential expression of a number of these genes was confirmed by QPCR (Table S2).
Figure 2
Figure 2
p16INK4a-deficiency induces a gene expression profile resembling IL-4-induced macrophage polarization
To further characterize this IL-4-like phenotype of p16−/− BMDM, the gene signature of these cells was compared with the gene signature of p16+/+ BMDM polarized in vitro by addition of IL-4 from day 0 of differentiation, generating p16+/+ AAM[var phi] [28]. Compared to p16+/+ BMDM, 14311 probesets were differentially expressed in p16+/+ AAM[var phi] (Figure 2C, green dots), whereas 7605 probesets were regulated in p16−/− BMDM (Figure 2C, red dots), of which the majority (78%) was also differentially expressed in p16+/+ AAM[var phi] (Figure 2C, blue dots). In addition, a strong correlation (p<0.0001; Pearson R=0.7; R2=0.5) was found between the two experimental conditions (Figure 2C), as also illustrated by a heat map representation of a selection of AAM[var phi] and CAM[var phi] marker genes (Figure 2D and Table S3).
Since p16−/− BMDM displayed lower expression levels of inflammatory genes (Figure 2A, D), the secretion of inflammatory cytokines produced in p16−/− BMDM compared to p16+/+ BMDM was measured. Under basal conditions, secretion of the pro-inflammatory cytokines IL-6 and TNF was lower (Figure 3A, B) in p16−/− BMDM. By contrast, secretion of anti-inflammatory IL-1Rn was, albeit modestly, higher (Figure 3C). These observations are in line with the microarray data and suggest that p16−/− BMDM are functionally different from their wild type counterparts.
Figure 3
Figure 3
p16INK4a-deficient macrophages phenotypically and functionally resemble IL-4-polarized alternatively activated macrophages
Next, we compared the response of p16−/− vs. p16+/+ BMDM to polarization into AAM[var phi] induced by IL-4 added at the start (day 0) of differentiation. Induction of the AAM[var phi] marker genes Arg-I (Figure 3D) and Ym1/2 (Figure 3E) was higher in p16−/− AAM[var phi]. However, induction of Mgl2 (Figure 3F) was not different in these cells, suggesting that the IL-4-responsiveness of certain, but not all, genes is dependent on p16INK4a. This heterogeneity in regulation of AAM[var phi] marker genes in IL-4-polarized p16−/− AAM[var phi] confirms the microarray results (Figure 2D).
Since p16−/− macrophages display increased AAM[var phi] marker expression after IL-4-induced polarization and since AAM[var phi] exert paracrine anti-inflammatory effects [29], the functional effects of p16INK4a-deficiency on IL-4-induced macrophage polarization were analyzed by indirect co-culture experiments. Hereto, conditioned medium from IL-4-polarized p16−/− or p16+/+ AAM[var phi] was added to p16+/+ BMDM and their response to LPS was measured (Figure 3G). Conditioned medium from p16−/− AAM[var phi] resulted in a more pronounced inhibition of LPS-induced secretion of IL-6 and TNF (Figure 3H, I). Thus, medium from p16−/− AAM[var phi] more potently inhibits pro-inflammatory responses.
Collectively, these results evidence that p16INK4a-deficiency results in a phenotype partially resembling IL-4-induced macrophage polarization. Moreover, IL-4-polarized p16−/− macrophages display a more pronounced AAM[var phi] phenotype.
p16INK4a-deficient macrophages are more responsive to IL-4, while they respond less to IFNγ or LPS
Since p16−/− BMDM resemble IL-4-polarized macrophages and since p16−/− AAM[var phi] show more potent anti-inflammatory effects than wild type macrophages, the response of p16−/− BMDM to acute (24h) IL-4 activation was assessed. Interestingly, IL-4 treatment resulted in a larger increase of Arg-I, Ym1/2 and Mgl2 mRNA in p16−/− compared to p16+/+ BMDM (Figure 4A–C). AAM[var phi] are known to be less sensitive to inflammatory stimuli [19]. Therefore, the effects of IFNγ and LPS, two pro-inflammatory stimuli, were tested on these cells. Interestingly, p16−/− BMDM were less responsive to IFNγ, shown by the lower induction of the IFNγ target genes iNOS, Cxcl10 and MHCII (Figure 4D–F), as well as to LPS, shown by the decreased response of the LPS-regulated genes TNF, IL-6 and MCP-1 (Figure 4G–I). Expression levels of the cognate receptors for IL-4, IFNγ and LPS was similar in both genotypes (Figure S4A–C), suggesting that the altered responses were not due to differences in receptor expression.
Figure 4
Figure 4
p16INK4a-deficiency modulates macrophage responses to alternatively and classically polarizing stimuli
Collectively, these data show that p16−/− BMDM are more responsive to alternative activation by IL-4 and less responsive to the classical macrophage activators IFNγ and LPS.
Haematopoietic p16INK4a-deficiency increases hepatic expression of alternatively activated macrophage markers upon S. mansoni infection
Since helminth parasite infections induce a strong Th2 immune response resulting in AAM[var phi] differentiation [20,30], the influence of p16INK4a-deficiency on macrophage polarization in vivo was investigated during S. mansoni infection. To assess the role of p16INK4a specifically in haematopoietic cells, p16+/+ and p16−/− bone marrow was transplanted in lethally irradiated wild type recipients. Mice were sacrificed 9 weeks after infection, corresponding to the peak of the Th2 immune response, and the hepatic pathology was subsequently characterized.
Expression of Th2 and Th1 cytokines in livers (Figure S5A–D) and spleens (Figure S6A–C), hepatic infection parameters (Table 1), plasma IgE levels (Figure S7), eosinophil infiltration (Table 1), as well as mortality and weight loss (data not shown) did not differ between p16−/− and p16+/+ transplanted animals. These results indicate that there are no differences in the lymphocyte-dependent Th2 response, in line with the very low expression of p16INK4a in T-cells (Figure 1A).
Table 1
Table 1
Liver pathology during Schistosomiasis
Since macrophages express significant levels of p16 INK4a (Figure 1A) and since these cells are abundant in S. mansoni-induced granulomas [20], macrophage markers were measured in the livers of infected mice. Hepatic mRNA levels of F4/80, CD68 and CD14 were equally induced upon infection (Figure 5A–C), indicating that macrophage numbers were not modified. However, the induction of the AAM[var phi] markers Ym1/2 (Figure 5D), Fizz1 (Figure 5E) and Mgl2 (Figure 5F) was higher in mice transplanted with p16−/− vs. p16+/+ bone marrow. Moreover, expression of the tissue remodeling markers αSMA and Timp1 (Fig. S5E, F) was higher in mice transplanted with p16−/− bone marrow, consistent with the tissue remodeling function of AAM[var phi] [31].
Figure 5
Figure 5
Haematopoietic deficiency of p16INK4a exacerbates hepatic alternative macrophage activation of S. mansoni-infected mice
Immunohistochemical analysis showed that the parasite-induced granulomas are highly macrophage-enriched (Figure S8). Moreover, Arg-I, Fizz1 and Ym1 co-localized with the general macrophage marker Moma-2. Surprisingly, the macrophage population within the granulomas appeared heterogeneous, since these markers did not entirely co-localize (Figure S8). Nevertheless, these data suggest that the increase in hepatic AAM[var phi] marker expression occurs mainly in macrophages. To unequivocally demonstrate this, the macrophage-positive areas of the granulomas were isolated by laser-capture micro-dissection from p16−/− and p16+/+ bone marrow transplanted mice and mRNA levels were measured. p16−/− granulomas displayed increased Mgl2 and Fizz1 mRNA levels, whereas Ym1/2 mRNA tended to be increased (Figure 5G–I). F4/80, CD68 and CD14 expression were identical, indicating that macrophage numbers did not differ between genotypes (data not shown).
Since macrophage polarization influences T-cell activation [20,32], the ex vivo response of splenocytes from mice transplanted with p16+/+ or p16−/− bone marrow to soluble S. mansoni egg antigen (SEA) was measured. Antigen-independent stimulation of naïve splenocytes by anti-CD3 showed similar IL-4 production (data not shown) suggesting an equal ability of T-cells to synthesize Th2 cytokines, regardless of macrophages within the splenocyte preparation. By contrast, antigen-dependent restimulation with SEA showed a lower production of both IL-4 and IFNγ in splenocytes from p16−/− transplanted mice (Figure S6D, E), while IL-10 production was similar (Figure S6F), hence resulting in an unchanged IL-4/IFNγ balance [33].
Collectively, these results provide evidence for a role of p16INK4a in AAM[var phi] skewing in vivo.
p16INK4-deficiency in macrophages decreases STAT1 and IKKα,β signaling without altering STAT6 phosphorylation
To unravel the mechanisms underlying the phenotype induced by p16INK4a-deficiency, the microarray data were analyzed to identify which pathways are affected. Interestingly, many genes with a decreased expression in p16−/− BMDM respond to activation of the IFNγ and NF-κB inflammatory signaling pathways (Figure S9), of which STAT1 and IKKα,β respectively are crucial components. Detailed examination of these gene expression patterns revealed that expression levels were comparable (Cxcl10, ifi27, ifi203, ifi47, ifit1, Ccl5, Irak3, Birc3 and Ly6e) or even lower (ifi44, CD55 and NFκBia) in p16−/− BMDM under basal conditions compared to IL-4-polarized p16+/+ AAM[var phi] (Figure 6). Moreover, most inflammatory genes were more strongly inhibited in IL-4-induced p16−/− AAM[var phi] than in p16+/+ AAM[var phi] (Figure 6 and Figure 2D), suggesting an additive effect of p16INK4a-deficiency on IL-4 treatment. By contrast, such a synergism could not be observed with respect to the AAM[var phi] marker genes since many of these AAM[var phi] marker genes responded similarly in IL-4-induced p16−/− and p16+/+ AAM[var phi] (Table S4 and Figure 2D). Collectively, these data show that the pathways controlling IFNγ, NF-κB, and IL-4 signaling are affected by p16INK4a-deficiency in macrophages.
Figure 6
Figure 6
p16INK4a-deficiency results in an alteration of STAT1 and NF-κB signaling
To determine whether the observed differences were related to indirect effects through pRb, BMDM were treated with CINK4, a potent inhibitor of pRb hyperphosphorylation [34]. CINK4 treatment resulted in a dose-dependent decrease of cyclin D mRNA levels both in p16+/+ and p16−/− BMDM (Figure S3). Furthermore, treatment with CINK4 in combination with IFNγ did not influence the different phenotype between the two genotypes (Figure S10), thus excluding a role for pRb therein.
STAT6 is the major transcription factor activated by IL-4. Surprisingly, IL-4 treatment induced STAT6 phosphorylation to a similar extent in p16−/− and p16+/+ BMDM (Figure 7A). By contrast, IFNγ-induced STAT1 phosphorylation (Figure 7B) and LPS-induced IKKα,β phosphorylation were markedly diminished (Figure 7C) in p16−/− vs. p16+/+ BMDM. Interestingly, IκBα protein levels were increased in p16−/− BMDM under basal conditions (Figure 7C). However, phosphorylation of p38, another downstream target of TLR-4, was not different between p16−/− and p16+/+ BMDM (Figure 7C), suggesting that p16INK4a-deficiency specifically alters the NF-κB response.
Figure 7
Figure 7
p16INK4a-deficiency diminishes JAK2-STAT1 and NF-κB signaling and increases acetylation of STAT1 and IKKα,β
Several genes coding for proteins with acetyl transferase activity were induced in p16−/− BMDM (Table 2). Acetylation of STAT1 and IKKα,β inhibits their phosphorylation and thereby their transcriptional activity [35,36]. Immunoprecipitation of acetylated proteins revealed that STAT1 and IKKα,β were acetylated to a higher extent in p16−/− than in p16+/+ BMDM (Figure 7D). To identify whether STAT1 acetylation is the cause or the consequence of decreased STAT1 phosphorylation, JAK2 phosphorylation, which is upstream in this pathway, was assessed. JAK2 phosphorylation was less pronounced under basal conditions and after activation with IFNγ in p16−/− BMDM (Figure 7E). Since acetylation of STAT1 can interfere with NF-κB signaling [36] and both pathways act synergistically [37], the decreased STAT1 and NF-κB signaling and their increased acetylation probably results from decreased JAK2 phosphorylation.
Table 2
Table 2
Genes coding for proteins with acetyl transferase activity in p16INK4a-deficient macrophages
We identify a novel role for the tumor suppressor protein p16INK4a in the regulation of the macrophage phenotype in vitro and in vivo. p16INK4a-deficiency promotes a STAT6-independent IL4-induced macrophage polarization, whereas LPS and IFNγ responses are lower. These actions of p16INK4a-deficiency likely occur through modification of the JAK2-STAT1 and NF-κB pathways,
Although p16INK4a is mainly known as a cell cycle inhibitor, cell cycle and macrophage maturation were unaffected in the absence of p16INK4a, and an E2F target gene signature[38,39], which would be expected to be increased by p16INK4a-deficiency, could not be identified in p16−/− BMDM. Since p15INK4b is a critical tumor suppressor in the absence of p16INK4a [40] and since an increase of p15INK4b expression was observed in p16−/− BMDM, a compensatory mechanism between these CDKI might have taken place with respect to cell cycle control.
Interestingly, p16INK4a has been previously shown to modulate transcriptional activities of the pro-inflammatory transcription factors NF-κB and AP-1. Via its ankyrin motifs, p16INK4a binds c-jun [41] and NF-κB [42], inhibiting their activity in several immortalized cell lines. However, this mechanism does not appear to play a role in primary murine macrophages, where the loss of p16INK4a has anti-inflammatory effects. Another CDKI, p21WAF1/CIP1, was also reported to modulate inflammation without altering cell cycle or differentiation. However, in contrast with p16INK4a-deficiency, p21WAF1/CIP1-deficiency in macrophages resulted in a higher sensitivity to inflammatory stimuli [43,44]. Additionally, p21WAF1/CIP1 expression was unchanged in p16−/− BMDM.
In a model of AAM[var phi] differentiation in vivo, infection with the helminth S. mansoni resulted in equal Th2-associated responses in p16−/− and p16+/+ bone marrow transplanted mice. These observations indicate unaltered T-lymphocyte function, in line with the low expression levels of p16INK4a in these cells. By contrast, AAM[var phi] markers were significantly increased in the livers and in hepatic granulomas of p16−/− bone marrow transplanted animals, probably due to a cell-autonomous activity of p16INK4a in macrophages. Since total bone marrow was transplanted, a contribution of other haematopoietic cell types to this cell-autonomous macrophage response cannot be excluded. However, since expression of the measured markers was also up-regulated in the macrophage-rich granulomas and since AAM[var phi] markers co-localized with macrophages in the granuloma, the effects are, at least in part, due to p16INK4a-deficiency in the macrophages. Surprisingly, different AAM[var phi] markers did not strictly co-localize, suggesting the existence of different macrophage populations in defined regions of the granuloma, which could be due to different gradients of stimuli within the granuloma.
Microarray analysis showed that p16−/− BMDM under basal conditions display a gene signature resembling that of IL-4-induced macrophage polarization [27], with the exception of the AAM[var phi] marker genes Ym1/2 and Fizz1. Moreover, p16−/− BMDM were more responsive to IL-4 activation and displayed weaker pro-inflammatory responses to IFNγ and LPS. Importantly, our data show that p16INK4a-deficiency does not influence pRb-mediated activation of the E2F transcription factor. The decreased IFNγ-induced phosphorylation of STAT1 and the LPS-induced IKKα,β phosphorylation in p16−/− BMDM probably account for the attenuated inflammatory responses. Decreased IKKα,β phosphorylation combined with increased IκBα protein levels correlated with the profound decrease of NF-κB target gene expression in p16−/− BMDM. Since a cluster of genes coding for proteins with acetyl transferase activity was induced in p16−/− BMDM and since STAT1 [36] and IKKα,β [35] acetylation reduces their ability to be phosphorylated, the decrease in STAT1 and IKKα,β phosphorylation may result from increased acetylation of these proteins in p16−/− BMDM. The acetylation-phosphorylation balance may be influenced by alterations upstream in the signaling pathway. Since phosphorylation of JAK2, the first component to be phosphorylated upon receptor dimerization [45], was decreased, it appears that the p16INK4a-deficiency-induced defect in JAK2 phosphorylation may be implicated in the reduced Stat1 phosphorylation. The increased acetylation status may be a consequence of this mechanism, contributing to the phenotype of p16−/− BMDM. Moreover, JAK2 phosphorylation was less pronounced already under basal culture conditions, in line with the observation that p16INK4a-deficiency confers a lower basal inflammatory phenotype, which is further exacerbated upon stimulation. Since p16INK4a-deficiency alters the IFNγ response early in the pathway and TLR4 signaling only at the level of NF-κB, but not, for example, at the level of p38, p16INK4a-deficiency thus likely acts directly on the IFNγ and indirectly on the NF-κB signaling pathway.
Surprisingly, STAT6 phosphorylation, the major transcription factor for IL-4-mediated signaling response, was comparable in BMDM of both genotypes, although IL-4-responsive genes were increased in p16−/− BMDM, suggesting that other pathways are involved. It has been shown that STAT1 activation antagonizes expression of STAT6-induced AAM[var phi] marker genes [46,47] and that decreased STAT1 phosphorylation can result in an increase of AAM[var phi] marker genes [48] by a number of molecular mechanisms. First, IL-4 action is inhibited by STAT1 activation through inhibition of STAT6 phosphorylation and its subsequent nuclear translocation in human monocytes [49]. However, p16INK4a-deficiency did not modify STAT6 phosphorylation. Second, IFNγ inhibits STAT6 activation by inducing the expression of the suppressor of cytokine signaling 1 (SOCS1) in macrophages [46]. Although SOCS1 mRNA levels were not different between p16−/− and p16+/+ BMDM (data not shown), we cannot exclude its involvement via post-transcriptional mechanisms. Third, STAT1 and STAT6 have been shown to compete for binding the same promoters [47], since decreased STAT1 activity increases binding of STAT6 to the promoters of several of its target genes. To our knowledge, an effect of NF-κB signaling on STAT6-dependent gene expression has not yet been demonstrated. Therefore, it is possible that the AAM[var phi]-like phenotype of p16−/− BMDM is secondary to the decreased CAM[var phi]-associated response via JAK2-STAT1.
In conclusion, our results identify p16INK4a as a novel modulator of macrophage polarization and show that p16INK4a-deficiency skews macrophages towards an IL-4-like phenotype. Since the CDKN2A locus is predictive for the risk of T2D and CVD [14,15], in which macrophage polarization plays a role [28,50], the role of p16INK4a in the control of macrophage function could be one mechanism contributing to the association of this locus with these diseases.
Figure S1: p16INK4a expression increases in F4/80+ cells during differentiation
mRNA expression of p16INK4a in wild type F4/80+ cells at different time points (d=day) during BMDM differentiation. Statistically significant differences compared to d4 are indicated (t-test; ***p<0.001 **p<0.01, and *p<0.05).
Figure S2: Compensatory increase of p15INK4b in p16−/− BMDM
mRNA expression of genes coding for proteins implicated in cell cycle control in p16+/+ (black) and p16−/− (white) BMDM. Statistically significant differences are indicated (t-test; ***p<0.001 **p<0.01, and *p<0.05).
Figure S3: CINK4 treatment dose-dependently inhibits Cyclin D expression
mRNA expression of cyclin D in p16+/+ (black) and p16−/−(white) BMDM treated with Cink4 at the indicated doses. Statistically significant differences are indicated (t-test; ***p<0.001 **p<0.01, and *p<0.05).
Figure S4: Receptor expression in p16−/− BMDM
mRNA expression from p16+/+and p16−/− BMDM. IL-4 receptor (A), IFNγ receptor I (B), and TLR-4 (C) was quantified by QPCR and expressed as fold increase compared to control.
Figure S5: Haematopoietic deficiency of p16INK4a does not modulate the immune response to parasite infection in the liver
Hepatic mRNA expression from mice transplanted with either p16+/+or p16−/− bone marrow which were not infected (naive) or infected with S. mansoni, 9 weeks post-infection. mRNA expression of the Th2 cytokines IL-4 (A), IL-10 (B), and IL-13 (C), the Th1 cytokine IFNγ (D) and of α SMA (E) and Timp1 (F) was quantified by QPCR and expressed as fold increase compared with their respective not infected controls. Data was obtained from n=10 naive and n=14 infected mice per genotype.
Figure S6: Haematopoietic deficiency of p16INK4a does not modulate the immune response to parasite infection in the spleen
Spleen mRNA expression from mice transplanted with either p16+/+or p16−/− bone marrow which were not infected (naive) or infected with S. mansoni, 9 weeks post-infection. mRNA expression of the Th2 cytokines IL-4 (A), IL-10 (B), and IL-13 (C) was quantified by QPCR and expressed as fold increase compared with their respective not infected controls. Data was obtained from n=10 naive and n=14 infected mice per genotype. (D–F) After splenocyte restimulation of isolated splenocytes from mice transplanted with either p16+/+or p16−/− bone marrow, protein secretion of IL-4 (D), IFNγ (E), and IL-10 (F) was measured in the supernatants of untreated controls and cells treated with SEA. Statistically significant differences are indicated (t-test; ***p<0.001 **p<0.01, and *p<0.05).
Figure S7: Haematopoietic deficiency of p16INK4a does not modulate the IgE level to parasite infection in plasma
Concentration of IgE in the plasma from mice transplanted with either p16+/+or p16−/− bone marrow and infected with S. mansoni, were measured by ELISA 9 weeks post-infection. Data was obtained from n=10 naive and n=14 infected mice per genotype
Figure S8: Co-localization of AAM[var phi] markers with macrophages in the granuloma
Representative immunostainings of macrophages (Moma-2) and the indicated AAM[var phi] markers (Arg-I, Fizz1, Ym1) within the same granuloma in adjacent slides of Schistosoma mansoni infected livers.
Figure S9: Genes downregulated in p16−/− BMDM cluster around NF-κB and STAT1
Network representation of genes lower expressed in p16−/− BMDM compared to p16+/+ BMDM, which are clustered around NF-κB and STAT1 (obtained using relative microarray intensity values and the Genomatix Bibliosphere® software). Genes regulated in our dataset are colored blue.
Figure S10: CINK4 treatment does not modulate the phenotype induced by p16INK4A-deficiency
mRNA expression of polarization marker genes in p16+/+ (black) and p16−/− (white) BMDM treated with 2.5μM Cink4 with or without IFNγ. Statistically significant differences compared to the corresponding wild type control are indicated (t-test; ***p<0.001 **p<0.01, and *p<0.05).
14
Acknowledgments
P. Krimpenfort provided p16INK4a-deficient mice. Discussions with G. Raes, J. Vanginderachter and M. de Winther are greatly acknowledged. We thank E. Vallez for mouse breeding, J. Brozek (Genfit SA, Loos, France) for microarray raw data analysis, T. Coevoet, N. Jouy and A. Lucas for technical assistance. This work was supported by the Fondation pour la Recherche Médicale (DCV20070409276 to B.S.), the EFSD/GSK Program 2009, the Cost Action (BM0602) and the Conseil régional Nord Pas-de-Calais and FEDER. C. Cudejko was supported by a doctoral fellowship from the Nouvelle Société Française d’Atherosclerose/Schering-Plough/MSD. K. Wouters was supported by a European FP7 Marie Curie grant (PIEF-GA-2009-235221) and a European Atherosclerosis Society grant.
The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
ABBREVIATIONS
AAM[var phi]Alternatively activated macrophage
BMDMBone marrow-derived macrophages
CAM[var phi]Classically activated macrophage
CDKCyclin-dependent kinase
CDKICyclin-dependent kinase inhibitor
DCDendritic cell
IFNγInterferon gamma
ILInterleukin
LPSLipopolysaccharide
p16−/−p16INK4a-deficient
p16+/+Wild type
QPCRQuantitative polymerase chain reaction
SEASoluble egg antigen
SOCS1Suppressor of cytokine signaling 1
STATSignal transducer and activator of transcription
T2DType 2 diabetes

Footnotes
Contributed by
C.C. and K.W. designed and performed experiments, analyzed data and wrote the manuscript. L.F., S.A.H., C.P., K.B., E.B., J.V., S.F. and P.R. contributed to some of the experiments. A.T. and G.C contributed to interpret data. D.D., B.S., R.P. contributed to interpretation of the data, manuscript preparation and project supervision. The authors declare no competing financial interests.
1. Serrano M, Hannon GJ, Beach D. A new regulatory motif in cell-cycle control causing specific inhibition of cyclin D/CDK4. Nature. 1993;366:704–7. [PubMed]
2. Hannon GJ, Beach D. p15INK4B is a potential effector of TGF-beta-induced cell cycle arrest. Nature. 1994;371:257–61. [PubMed]
3. Guan KL, Jenkins CW, Li Y, Nichols MA, Wu X, O’Keefe CL, Matera AG, Xiong Y. Growth suppression by p18, a p16INK4/MTS1- and p14INK4B/MTS2-related CDK6 inhibitor, correlates with wild-type pRb function. Genes Dev. 1994;8:2939–52. [PubMed]
4. Chan FK, Zhang J, Cheng L, Shapiro DN, Winoto A. Identification of human and mouse p19, a novel CDK4 and CDK6 inhibitor with homology to p16ink4. Mol Cell Biol. 1995;15:2682–8. [PMC free article] [PubMed]
5. Hirai H, Roussel MF, Kato JY, Ashmun RA, Sherr CJ. Novel INK4 proteins, p19 and p18, are specific inhibitors of the cyclin D-dependent kinases CDK4 and CDK6. Mol Cell Biol. 1995;15:2672–81. [PMC free article] [PubMed]
6. Sharpless NE. INK4a/ARF: a multifunctional tumor suppressor locus. Mutat Res. 2005;576:22–38. [PubMed]
7. Alcorta DA, Xiong Y, Phelps D, Hannon G, Beach D, Barrett JC. Involvement of the cyclin-dependent kinase inhibitor p16 (INK4a) in replicative senescence of normal human fibroblasts. Proc Natl Acad Sci US A. 1996;93:13742–7. [PubMed]
8. Hara E, Smith R, Parry D, Tahara H, Stone S, Peters G. Regulation of p16CDKN2 expression and its implications for cell immortalization and senescence. Mol Cell Biol. 1996;16:859–67. [PMC free article] [PubMed]
9. Krishnamurthy J, Torrice C, Ramsey MR, Kovalev GI, Al-Regaiey K, Su L, Sharpless NE. Ink4a/Arf expression is a biomarker of aging. J Clin Invest. 2004;114:1299–307. [PMC free article] [PubMed]
10. Nielsen GP, Stemmer-Rachamimov AO, Shaw J, Roy JE, Koh J, Louis DN. Immunohistochemical survey of p16INK4A expression in normal human adult and infant tissues. Lab Invest. 1999;79:1137–43. [PubMed]
11. Zindy F, Quelle DE, Roussel MF, Sherr CJ. Expression of the p16INK4a tumor suppressor versus other INK4 family members during mouse development and aging. Oncogene. 1997;15:203–11. [PubMed]
12. Melzer D, Frayling TM, Murray A, Hurst AJ, Harries LW, Song H, Khaw K, Luben R, Surtees PG, Bandinelli SS, Corsi A, Ferrucci L, Guralnik JM, Wallace RB, Hattersley AT, Pharoah PD. A common variant of the p16(INK4a) genetic region is associated with physical function in older people. Mech Ageing Dev. 2007;128:370–7. [PMC free article] [PubMed]
13. Janzen V, Forkert R, Fleming HE, Saito Y, Waring MT, Dombkowski DM, Cheng T, DePinho RA, Sharpless NE, Scadden DT. Stem-cell ageing modified by the cyclin-dependent kinase inhibitor p16INK4a. Nature. 2006;443:421–6. [PubMed]
14. McPherson R, Pertsemlidis A, Kavaslar N, Stewart A, Roberts R, Cox DR, Hinds DA, Pennacchio LA, Tybjaerg-Hansen A, Folsom AR, Boerwinkle E, Hobbs HH, Cohen JC. A common allele on chromosome 9 associated with coronary heart disease. Science. 2007;316:1488–91. [PMC free article] [PubMed]
15. Liu Y, Sanoff HK, Cho H, Burd CE, Torrice C, Mohlke KL, Ibrahim JG, Thomas NE, Sharpless NE. INK4/ARF transcript expression is associated with chromosome 9p21 variants linked to atherosclerosis. PLoS One. 2009;4:e5027. [PMC free article] [PubMed]
16. Saxena R, Voight BF, Lyssenko V, Burtt NP, de Bakker PIW, Chen H, Roix JJ, Kathiresan S, Hirschhorn JN, Daly MJ, Hughes TE, Groop L, Altshuler D, Almgren P, Florez JC, Meyer J, Ardlie K, Bengtsson Boström K, Isomaa B, Lettre G, Lindblad U, Lyon HN, Melander O, Newton-Cheh C, Nilsson P, Orho-Melander M, Råstam L, Speliotes EK, Taskinen M, Tuomi T, Guiducci C, Berglund A, Carlson J, Gianniny L, Hackett R, Hall L, Holmkvist J, Laurila E, Sjögren M, Sterner M, Surti A, Svensson M, Svensson M, Tewhey R, Blumenstiel B, Parkin M, Defelice M, Barry R, Brodeur W, Camarata J, Chia N, Fava M, Gibbons J, Handsaker B, Healy C, Nguyen K, Gates C, Sougnez C, Gage D, Nizzari M, Gabriel SB, Chirn G, Ma Q, Parikh H, Richardson D, Ricke D, Purcell S. Genome-wide association analysis identifies loci for type 2 diabetes and triglyceride levels. Science. 2007;316:1331–6. [PubMed]
17. Wei S, Lightwood D, Ladyman H, Cross S, Neale H, Griffiths M, Adams R, Marshall D, Lawson A, McKnight AJ, Stanley ER. Modulation of CSF-1-regulated post-natal development with anti-CSF-1 antibody. Immunobiology. 2005;210:109–19. [PubMed]
18. Baffy G. Kupffer cells in non-alcoholic fatty liver disease: the emerging view. J Hepatol. 2009;51:212–23. [PMC free article] [PubMed]
19. Gordon S. Alternative activation of macrophages. Nat Rev Immunol. 2003;3:23–35. [PubMed]
20. Herbert DR, Hölscher C, Mohrs M, Arendse B, Schwegmann A, Radwanska M, Leeto M, Kirsch R, Hall P, Mossmann H, Claussen B, Förster I, Brombacher F. Alternative macrophage activation is essential for survival during schistosomiasis and downmodulates T helper 1 responses and immunopathology. Immunity. 2004;20:623–35. [PubMed]
21. Bellosta S, Via D, Canavesi M, Pfister P, Fumagalli R, Paoletti R, Bernini F. HMG-CoA reductase inhibitors reduce MMP-9 secretion by macrophages. Arterioscler Thromb Vasc Biol. 1998;18:1671–8. [PubMed]
22. Dubois A, Deruytter N, Adams B, Kanda A, Delbauve S, Fleury S, Torres D, François A, Pétein M, Goldman M, Dombrowicz D, Flamand V. Regulation of Th2 Responses and Allergic Inflammation through Bystander Activation of CD8+ T Lymphocytes in Early Life. J Immunol. 2010 [PubMed]
23. Van Ginderachter JA, Movahedi K, Hassanzadeh Ghassabeh G, Meerschaut S, Beschin A, Raes G, De Baetselier P. Classical and alternative activation of mononuclear phagocytes: picking the best of both worlds for tumor promotion. Immunobiology. 2006;211:487–501. [PubMed]
24. Vats D, Mukundan L, Odegaard JI, Zhang L, Smith KL, Morel CR, Wagner RA, Greaves DR, Murray PJ, Chawla A. Oxidative metabolism and PGC-1beta attenuate macrophage-mediated inflammation. Cell Metab. 2006;4:13–24. [PMC free article] [PubMed]
25. Martinez FO, Gordon S, Locati M, Mantovani A. Transcriptional profiling of the human monocyte-to-macrophage differentiation and polarization: new molecules and patterns of gene expression. J Immunol. 2006;177:7303–11. [PubMed]
26. Noël W, Raes G, Hassanzadeh Ghassabeh G, De Baetselier P, Beschin A. Alternatively activated macrophages during parasite infections. Trends Parasitol. 2004;20:126–33. [PubMed]
27. Mantovani A, Sica A, Sozzani S, Allavena P, Vecchi A, Locati M. The chemokine system in diverse forms of macrophage activation and polarization. Trends Immunol. 2004;25:677–86. [PubMed]
28. Bouhlel MA, Derudas B, Rigamonti E, Dièvart R, Brozek J, Haulon S, Zawadzki C, Jude B, Torpier G, Marx N, Staels B, Chinetti-Gbaguidi G. PPARgamma activation primes human monocytes into alternative M2 macrophages with anti-inflammatory properties. Cell Metab. 2007;6:137–43. [PubMed]
29. Katakura T, Miyazaki M, Kobayashi M, Herndon DN, Suzuki F. CCL17 and IL-10 as effectors that enable alternatively activated macrophages to inhibit the generation of classically activated macrophages. J Immunol. 2004;172:1407–13. [PubMed]
30. Pearce EJ, Kane MC, Sun J, Taylor JJ, McKee AS, Cervi L. Th2 response polarization during infection with the helminth parasite Schistosoma mansoni. Immunol Rev. 2004;201:117–26. [PubMed]
31. Wynn TA. Fibrotic disease and the T(H)1/T(H)2 paradigm. Nat Rev Immunol. 2004;4:583–94. [PMC free article] [PubMed]
32. Elliott DE, Boros DL. Schistosome egg antigen(s) presentation and regulatory activity by macrophages isolated from vigorous or immunomodulated liver granulomas of Schistosoma mansoni-infected mice. J Immunol. 1984;132:1506–10. [PubMed]
33. Mosmann TR, Coffman RL. TH1 and TH2 cells: different patterns of lymphokine secretion lead to different functional properties. Annu Rev Immunol. 1989;7:145–73. [PubMed]
34. Soni R, O’Reilly T, Furet P, Muller L, Stephan C, Zumstein-Mecker S, Fretz H, Fabbro D, Chaudhuri B. Selective in vivo and in vitro effects of a small molecule inhibitor of cyclin-dependent kinase 4. J Natl Cancer Inst. 2001;93:436–46. [PubMed]
35. Mittal R, Peak-Chew S, McMahon HT. Acetylation of MEK2 and I kappa B kinase (IKK) activation loop residues by YopJ inhibits signaling. Proc Natl Acad Sci US A. 2006;103:18574–9. [PubMed]
36. Krämer OH, Baus D, Knauer SK, Stein S, Jäger E, Stauber RH, Grez M, Pfitzner E, Heinzel T. Acetylation of Stat1 modulates NF-kappaB activity. Genes Dev. 2006;20:473–85. [PubMed]
37. Hiroi M, Ohmori Y. The transcriptional coactivator CREB-binding protein cooperates with STAT1 and NF-kappa B for synergistic transcriptional activation of the CXC ligand 9/monokine induced by interferon-gamma gene. J Biol Chem. 2003;278:651–60. [PubMed]
38. Vernell R, Helin K, Müller H. Identification of target genes of the p16INK4A-pRB- E2F pathway. J Biol Chem. 2003;278:46124–37. [PubMed]
39. Stanelle J, Stiewe T, Theseling CC, Peter M, Pützer BM. Gene expression changes in response to E2F1 activation. Nucleic Acids Res. 2002;30:1859–67. [PMC free article] [PubMed]
40. Krimpenfort P, Ijpenberg A, Song J, van der Valk M, Nawijn M, Zevenhoven J, Berns A. p15Ink4b is a critical tumour suppressor in the absence of p16Ink4a. Nature. 2007;448:943–6. [PubMed]
41. Choi BY, Choi HS, Ko K, Cho Y, Zhu F, Kang BS, Ermakova SP, Ma W, Bode AM, Dong Z. The tumor suppressor p16(INK4a) prevents cell transformation through inhibition of c-Jun phosphorylation and AP-1 activity. Nat Struct Mol Biol. 2005;12:699–707. [PubMed]
42. Wolff B, Naumann M. INK4 cell cycle inhibitors direct transcriptional inactivation of NF-kappaB. Oncogene. 1999;18:2663–6. [PubMed]
43. Scatizzi JC, Mavers M, Hutcheson J, Young B, Shi B, Pope RM, Ruderman EM, Samways DSK, Corbett JA, Egan TM, Perlman H. The CDK domain of p21 is a suppressor of IL-1beta-mediated inflammation in activated macrophages. Eur J Immunol. 2009;39:820–5. [PMC free article] [PubMed]
44. Trakala M, Arias CF, García MI, Moreno-Ortiz MC, Tsilingiri K, Fernández PJ, Mellado M, Díaz-Meco MT, Moscat J, Serrano M, Martínez-A C, Balomenos D. Regulation of macrophage activation and septic shock susceptibility via p21(WAF1/CIP1) Eur J Immunol. 2009;39:810–9. [PubMed]
45. Shuai K, Liu B. Regulation of JAK-STAT signalling in the immune system. Nat Rev Immunol. 2003;3:900–11. [PubMed]
46. Dickensheets HL, Venkataraman C, Schindler U, Donnelly RP. Interferons inhibit activation of STAT6 by interleukin 4 in human monocytes by inducing SOCS-1 gene expression. Proc Natl Acad Sci US A. 1999;96:10800–5. [PubMed]
47. Ohmori Y, Hamilton TA. IL-4-induced STAT6 suppresses IFN-gamma-stimulated STAT1-dependent transcription in mouse macrophages. J Immunol. 1997;159:5474–82. [PubMed]
48. Porta C, Rimoldi M, Raes G, Brys L, Ghezzi P, Di Liberto D, Dieli F, Ghisletti S, Natoli G, De Baetselier P, Mantovani A, Sica A. Tolerance and M2 (alternative) macrophage polarization are related processes orchestrated by p50 nuclear factor kappaB. Proc Natl Acad Sci US A. 2009;106:14978–83. [PubMed]
49. Dickensheets HL, Donnelly RP. Inhibition of IL-4-inducible gene expression in human monocytes by type I and type II interferons. J Leukoc Biol. 1999;65:307–12. [PubMed]
50. Odegaard JI, Ricardo-Gonzalez RR, Goforth MH, Morel CR, Subramanian V, Mukundan L, Red Eagle A, Vats D, Brombacher F, Ferrante AW, Chawla A. Macrophage-specific PPARgamma controls alternative activation and improves insulin resistance. Nature. 2007;447:1116–20. [PMC free article] [PubMed]