Published in Volume
120, Issue 1
(January 4, 2010)J Clin Invest.
Copyright © 2010, American Society for Clinical Investigation
Stat3-dependent acute Rantes production in vascular smooth muscle cells modulates inflammation following arterial injury in mice
1Translational Medicine Branch, National Heart, Lung, and Blood Institute, NIH, Bethesda, Maryland, USA.
2Genome Technology Branch, National Human Genome Research Institute, NIH, Bethesda, Maryland, USA.
Address correspondence to: Manfred Boehm, Building 10-CRC, Room 5-3132, Translational Medicine Branch, National Heart, Lung, and Blood Institute, National Institutes of Health, Bethesda, Maryland 20892, USA. Phone: (301) 435-7211; Fax: (301) 451-7090; E-mail:
First published December 28, 2009
Submitted: July 1,
2009; Accepted: October 7,
Inflammation is a key component of arterial injury, with VSMC proliferation and neointimal formation serving as the final outcomes of this process. However, the acute events transpiring immediately after arterial injury that establish the blueprint for this inflammatory program are largely unknown. We therefore studied these events in mice and found that immediately following arterial injury, medial VSMCs upregulated Rantes in an acute manner dependent on Stat3 and NF-κB (p65 subunit). This led to early T cell and macrophage recruitment, processes also under the regulation of the cyclin-dependent kinase inhibitor p21Cip1. Unique to VSMCs, Rantes production was initiated by Tnf-α, but not by Il-6/gp130. This Rantes production was dependent on the binding of a p65/Stat3 complex to NF-κB–binding sites within the Rantes promoter, with shRNA knockdown of either Stat3 or p65 markedly attenuating Rantes production. In vivo, acute NF-κB and Stat3 activation in medial VSMCs was identified, with acute Rantes production after injury substantially reduced in Tnfa–/– mice compared with controls. Finally, we generated mice with SMC-specific conditional Stat3 deficiency and confirmed the Stat3 dependence of acute Rantes production by VSMCs. Together, these observations unify inflammatory events after vascular injury, demonstrating that VSMCs orchestrate the arterial inflammatory response program via acute Rantes production and subsequent inflammatory cell recruitment.
Inflammation, cytokine production, and VSMC proliferation are pivotal aspects of arterial wound repair (1, 2). Unfortunately, this process often culminates in excessive neointimal formation and decreased luminal diameter (1, 2), a pathology associated with adverse clinical outcomes (3). Although early inflammation is known to modulate this process (4), given the clinical implications of reduced luminal diameter (3), investigators have generally chosen to focus on late events surrounding neointimal formation and VSMC proliferation. Conversely, significantly less attention has been paid to the acute immune responses that orchestrate the initial vascular inflammatory response program and establish the blueprint for vascular repair.
An additional key component of this process is the recruitment of macrophages and T cells (1, 2, 5). While certain regulatory subtypes differ in their responses (6, 7), macrophage and T cell recruitment typically leads to enhanced inflammation and neointimal formation as well as reduced luminal patency (1, 2, 5, 8–11). A complex network of cytokines, chemokines, and their receptors is known to regulate recruitment of these cells (2, 5, 10–14). However, surprisingly little data are available regarding acute local cytokine/chemokine production or early vascular inflammatory cell infiltration.
We recently identified increased T cell and macrophage infiltration and enhanced neointimal formation 1 and 2 weeks after arterial injury in p21–/– compared with WT mice (2). These findings were related to enhanced Stat3 activity in p21–/– VSMCs (2) and are consistent with reports indicating that p21Cip1 inhibits Stat3-mediated gene transcription (15) and that Stat3 is an important inflammatory mediator (16, 17). Of relevance, at least in epithelial cells, Stat3 may form a transcription complex with NF-κB, another key inflammatory mediator (18), leading to the expression of Rantes (17).
Rantes, otherwise known as Ccl5, is a chemokine produced in response to stimulation by cytokines such as Il-6 (17) and/or Tnf-α (19) and may be secreted by a variety of cells, including VSMCs (14, 20), epithelial cells (17), T cells (21), macrophages (22), and also platelets (14, 23). Rantes exerts a multitude of generally proinflammatory effects and is of importance in T cell and monocyte chemoattraction (24), T cell proliferation, and the delayed-type hypersensitivity response (25). Correspondingly, Rantes may be involved in the pathobiology of several clinical inflammatory conditions, such as cardiac allograft vasculopathy (21), atherosclerosis (26, 27), asthma (28), and rheumatoid arthritis (29).
While Rantes is clearly implicated in the vascular response to injury, the majority of prior studies considered only long-term actions and effects over the duration of vascular healing (14, 20, 23, 27, 30, 31). The role of Rantes in the acute phase of vascular injury and the potential interrelationships of p21Cip1 and Rantes signaling are virtually unexplored. Here, we characterize early events surrounding initiation of the vascular inflammatory response program, which is notable for a striking upregulation of Rantes production by VSMCs. Synthesis of Rantes by VSMCs occurs in response to Tnf-α and downstream binding of a complex formed between NF-κB (p65 subunit) and Stat3 to the Rantes promoter, which is restrained by p21Cip1 and independent of the Il-6/gp130 pathway. This NF-κB/Stat3/Rantes signaling pathway orchestrates early T cell and macrophage recruitment, thereby identifying VSMCs as exerting an immune-modulating role during the acute response to vascular injury.
Acute T cell and macrophage recruitment following arterial wire injury. We examined inflammatory cell recruitment after femoral artery injury in WT mice and identified an acute infiltration of macrophages and T cells. From baseline (uninjured) to 1 day after injury, CD3+ T cells increased approximately 20-fold from 0.5% ± 0.3% (n = 9) to 9.7% ± 1.7% (n = 10) of all vessel-associated cells (P < 0.0001) (Figure 1 and Supplemental Figure 1; supplemental material available online with this article; doi:
10.1172/JCI40364DS1). Relative T cell infiltration plateaued 1 to 3 days after injury and subsequently declined, decreasing from 10.3% ± 2.4% (n = 8) at 3 days to 4.0% ± 1.0% (n = 10) by 7 days after injury (P < 0.05) (Figure 1). In contrast, acute CD115+ macrophage infiltration was somewhat less pronounced, increasing from 4.7% ± 0.7% (n = 8) to 8.5% ± 1.1% (n = 10) (uninjured versus 1 day after injury; P < 0.05). However, macrophage recruitment was ongoing, with relative infiltration peaking 3 days after injury in WT mice at 29.6% ± 4.3% (n = 9) (Supplemental Figures 2 and 3). To validate these observations, we employed a second animal model, utilizing mice with genetic p21Cip1 deletion, which are known to exhibit enhanced inflammation following arterial injury (2, 32, 33). We found that p21–/– mice displayed augmented early CD3+ T cell recruitment, with CD3+ T cells representing 22.9% ± 2.6 % (n = 7) of all vessel-associated cells 1 day after injury in p21–/– mice (p21–/– versus WT; P < 0.001) (Figure 1 and Supplemental Figure 1). Although absolute numbers of infiltrating CD3+ T cells and CD115+ macrophages were consistently higher in p21–/– versus WT mice after injury (Supplemental Figure 4, A and B), unlike T cells, the percentage of macrophages at both 3 and 14 days after injury was identical in WT and p21–/– mice (Supplemental Figure 2). Consistent with prior reports (34, 35), we also identified a marked loss of medial VSMCs following arterial injury (Supplemental Figure 4C). To further confirm these findings, we examined CD3 and CD115 mRNA levels in femoral artery sections harvested uninjured or after vascular injury. Consistent with our other data (above), we identified a progressive and p21Cip1-dependent increase in the mRNA levels of both genes following vascular injury (Supplemental Figure 5). Collectively, these data demonstrate that arterial injury results in a marked acute and p21Cip1-regulated local CD3+ T cell infiltration, with a more delayed infiltration observed for CD115+ macrophages.
CD3+ T cell infiltration following arterial wire injury.
(A) Relative CD3+ T cell infiltration in WT and p21–/– mice. Data are shown as mean ± SEM. (B) Representative corresponding confocal microscopic images of femoral artery sections showing CD3+ T cells (green) in uninjured vessels and at 6 hours and 1 day following arterial wire injury, with the dashed square indicating an area of higher magnification shown in the upper-right corner for the 1-day images. Width of inset square: 70 μm. Nuclei (blue) were stained with DAPI. Arterial elastic laminae are visible in green due to autofluorescence. Scale bars: 100 μm.
Acute Rantes, p21Cip1, and Stat3 expression by VSMCs after arterial injury.
Based on the above observations, we examined local vascular expression of Rantes, a known T cell and macrophage chemoattractant (24), revealing acute local upregulation of Rantes mRNA expression within 6 hours of injury (Figure 2A). Consistent with the enhanced p21–/– vascular inflammatory response (2, 32, 33) and pattern of CD3+ cell infiltration, local Rantes expression 3 and 6 hours after injury was greater in p21–/– than WT mice. Although local vascular Rantes levels also trended higher in p21–/– versus WT mice at 12 hours, 1 day, and 3 days after injury, perhaps related to concurrent medial VSMC loss (Supplemental Figure 4C), these differences were not significant (Figure 2A). Local expression levels of other potential acute T cell chemoattractants after vascular injury, while at times increased, were less marked than that of Rantes and not consistent with the pattern of early T cell infiltration (Supplemental Figure 6).
Rantes production is acutely upregulated following arterial injury and produced locally by medial VSMCs. (A) Local Rantes (left panel), p21Cip1 (middle panel), and Stat3 (right panel) mRNA expression after arterial injury by qRT-PCR. Comparisons shown are WT versus p21–/– at each respective time point for Rantes and Stat3, with p21Cip1 expression assessed in WT mice only. *P < 0.05; **P < 0.01; ***P < 0.0001. Also, in WT mice from baseline (uninjured) to 6 hours after injury, local vascular Rantes mRNA expression increased 21-fold (n = 5 both groups; P < 0.05); p21Cip1 mRNA expression increased 58-fold (n = 10 at baseline, n = 7 at 6 hours; P < 0.005); and Stat3 mRNA expression increased 3.5-fold (n = 7 at baseline, n = 12 at 6 hours; P < 0.001). (B) Representative confocal microscopic images of Rantes immunofluorescence staining of femoral artery sections from WT mice at baseline (uninjured) and 6 hours after injury. Rantes is shown in red, nuclei in blue (DAPI). Arterial elastic laminae are visible in green due to autofluorescence. Scale bars: 100 μm. (C) BM-transplanted mice were used to localize Rantes production 6 hours after arterial injury. By ANOVA (overall P = 0.0045), Rantes–/– mice reconstituted with WT BM (WT to Rantes–/–; n = 4) had decreased femoral artery Rantes mRNA expression in comparison with WT mice reconstituted with either WT (WT to WT, n = 6; *P < 0.05 versus WT to Rantes–/–) or Rantes–/– BM (Rantes–/– to WT, n = 5; *P < 0.05 versus WT to Rantes–/–). Data are shown as mean + SEM.
Local vascular mRNA expression of p21Cip1 and Stat3 also increased acutely after injury (Figure 2A). Interestingly, the pattern and time course of increased p21Cip1 expression corresponded to that of both Rantes and Stat3, reinforcing our finding that Rantes expression is greater in p21–/– than WT mice, but also suggesting that p21Cip1 may modulate Stat3 transcription. Indeed, including at 6 hours after injury, Stat3 mRNA expression in injured vessels was generally 1- to 4-fold higher in p21–/– than WT mice (Figure 2A). We further validated these in vivo data by examining Rantes and Stat3 levels in vitro in VSMCs. These studies confirmed increased Rantes mRNA (Supplemental Figure 7A) and protein (Supplemental Figure 7B) expression in p21–/– versus WT VSMCs. Similarly, Stat3 mRNA expression was also greater in p21–/– versus WT VSMCs (Supplemental Figure 7C), with the magnitude of increased Stat3 expression in p21–/– versus WT (~2.5-fold) consistent between our in vitro and in vivo studies.
Confocal immunofluorescence microscopy was used to localize the site of acute Rantes production. While occasional adventitial cells stained positive for Rantes, overwhelmingly, the greatest positive Rantes staining was in medial VSMCs (Figure 2B). We verified that increased Rantes mRNA levels after injury were due to enhanced local production, and not infiltrating BM cells, by reciprocal BM transplantation between WT and Rantes–/– mice. These experiments confirmed that more than 70% of Rantes in vessels 6 hours after injury was locally derived, while less than 30% potentially arose from BM-derived cells (Figure 2C).
Vascular Rantes expression regulates inflammatory cell infiltration and neointimal formation following arterial injury. To investigate the functional role of acute Rantes production by medial VSMCs, we examined inflammatory cell infiltration at 1 day after injury in WT and Rantes–/– mice reconstituted with WT BM (WT to WT and WT to Rantes–/–, respectively). As expected, CD3+ T cell and CD115+ macrophage infiltration 1 day after injury were similar between WT to WT mice (Figure 3, A and B) and our original experiments using WT mice without BM transplantation (Figure 1A and Supplemental Figure 2A). However, compared with WT to WT, WT to Rantes–/– mice displayed a marked reduction in CD3+ T cell and CD115+ macrophage infiltration (Figure 3, A and B, and Supplemental Figure 8), indicating that acute local Rantes production regulates early T cell and macrophage recruitment following arterial injury.
Local vascular Rantes production regulates early CD3+ T cell and CD115+ macrophage infiltration and late neointimal formation following arterial injury.
(A) WT to WT and WT to Rantes–/– mice underwent arterial injury, and cell infiltration was assessed at 1 day. Relative CD3+ T cell infiltration was reduced in WT to Rantes–/– mice compared with WT to WT mice (n = 6 for WT to WT, n = 9 for WT to Rantes–/–; ****P < 0.0005). (B) Relative CD115+ macrophage infiltration was reduced 1 day after arterial injury in WT to Rantes–/– mice compared with WT to WT mice (n = 7 for WT to WT, n = 9 for WT to Rantes–/–; ****P < 0.0005). (C) Neointimal formation at 3 weeks after arterial injury, as assessed by intima/media ratio, was decreased in femoral vessels from WT to Rantes–/– as compared with WT to WT mice (n = 9 for WT to WT, n = 8 for WT to Rantes–/–; **P < 0.001). Data are shown as mean + SEM. (D) Representative cross sections of femoral arteries from WT to WT and WT to Rantes mice at 3 weeks after arterial wire injury (stained with H&E). Arrows indicate the internal elastic lamina. Scale bars: 100 μm.
Systemic Rantes antagonism is associated with reduced neointimal formation after vascular injury (14). However, the relative contributions of local vascular Rantes production versus BM cell– and platelet–derived Rantes to augmented neointimal formation are unknown. Therefore, WT to WT and WT to Rantes–/– mice were subjected to arterial wire injury, and neointimal formation was assessed after 3 weeks. Consistent with the concept that local Rantes production modulates the vascular inflammatory response program, neointimal formation in WT to Rantes–/– mice was significantly reduced compared with that in WT to WT mice (Figure 3, C and D).
NF-κB and Stat3 interact to modulate Rantes transcriptional activity in VSMCs. We sought to identify early p65 and Stat3 activation in medial VSMCs — transcription factors known to regulate Rantes production (17, 36). In uninjured vessels, consistent with prior reports (37, 38), we identified p65 and Stat3 cytoplasmic staining in endothelial cells. However, p65, Stat3, and phosphorylated Stat3 (p-Stat3) were not detectable in medial VSMCs from uninjured vessels (Figure 4). Within hours of arterial injury (and endothelial denudation), endothelial staining for these proteins was absent, but robust perinuclear and nuclear staining for p65, Stat3, and p-Stat3 were apparent in the medial VSMC layer (Figure 4), indicating early NF-κB and Stat3 activation in VSMCs and suggesting these transcription factors may play a role in acute Rantes production.
Stat3 and p65 are acutely activated following arterial injury in medial VSMCs. Representative confocal images of immunofluorescence-stained femoral artery sections from WT mice at baseline (uninjured) and acutely after injury for p65 (6 hours after injury), Stat3 (6 hours after injury), and p-Stat3 (Tyr705) (3 hours after injury). p65, Stat3, and p-Stat3 are shown in red, nuclei in blue (DAPI). Arterial elastic laminae are visible in green due to autofluorescence. Scale bars: 20 μm.
We then interrogated the murine Rantes promoter and identified 2 likely NF-κB–binding sites. These sites spanned –372 to –363 (NF-κB–binding site no. 1) and –88 to –77 (NF-κB–binding site no. 2) of the Rantes promoter, with at least 1 site (no. 2) previously identified and validated in 3T3 fibroblasts (36). We mutated both putative NF-κB–binding sites in a luciferase plasmid containing the murine Rantes promoter and individually transfected mutated (M1 and M2) and nonmutated luciferase control (Co) constructs into WT and p21–/– VSMCs. In Co VSMCs, consistent with Rantes expression and secretion, Rantes promoter activity was increased in p21–/– versus WT VSMCs (Figure 5A). Furthermore, mutation of either putative NF-κB–binding site markedly reduced Rantes promoter activity (Figure 5A).
Stat3 and p65 coassociate and regulate Rantes expression in VSMCs. (A) VSMCs were transfected with reporter plasmids containing the native Rantes promoter (Co) or mutated plasmids (M1 or M2) designed to abolish putative NF-κB–binding site activity. Location and sequence of putative NF-κB–binding sites and mutations are indicated. Comparisons are Co p21–/– versus Co WT, or M1 or M2 versus Co for WT and p21–/–. pGL2 indicates WT VSMCs transfected with pGL2 plasmid containing no promoter. n = 3 for all groups; **P < 0.005, ***P < 0.001, ****P < 0.0001. (B) shRNA p65Kd in p21 VSMCs reduced mRNA expression of p65 (left panel, n = 3 both groups; **P < 0.01) and Rantes (right panel, n = 4 both groups; *P < 0.05) compared with Co shRNA. (C) Tnf-α treatment for 4 hours increased Rantes mRNA expression in WT Co VSMCs (n = 6 for unstimulated, n = 7 for stimulated; P < 0.0005), while p65Kd and Stat3Kd VSMCs exhibited attenuated Tnf-α–induced Rantes mRNA expression compared with Tnf-α–treated Co VSMCs (p65Kd: n = 3, *P < 0.05; Stat3Kd: n = 4, **P < 0.005). Data are shown as mean + SEM. (D) IP followed by WB in WT Co and Stat3Kd VSMCs (input protein levels as indicated). IP with anti-Stat3 then WB with anti-p65 (upper left) and IP with anti-p65 then WB with anti-Stat3 (lower left) revealed coassociation of p65 and Stat3. IP with anti-p65 then WB with anti-p21Cip1 (upper right) revealed coassociation of p65 with p21Cip1, which was virtually abolished in Stat3Kd VSMCs.
To confirm that NF-κB is required for VSMC Rantes transcription and considering the increased Rantes expression in p21–/– versus WT VSMCs, we performed targeted NF-κB knockdown by transfecting p21–/– VSMCs with either shRNA directed against p65 (p65 knockdown [p65Kd]) or Co shRNA. These studies verified that disturbed NF-κB signaling is associated with reduced Rantes mRNA expression in VSMCs (Figure 5B).
Similarly, based on our above-mentioned findings and reports in other cell types (17), we speculated that Stat3 may mediate Rantes transcription in VSMCs. Thus, both p65Kd and Stat3 knockdown (Stat3Kd) were performed in WT VSMCs (Supplemental Figure 9, A–C). We noted that Co WT VSMCs exhibit increased Rantes mRNA expression in response to Tnf-α (Figure 5C). However, following Tnf-α treatment, Rantes mRNA expression was markedly attenuated in both p65Kd and Stat3Kd VSMCs compared with Tnf-α–treated Co VSMCs (Figure 5C).
To explore the possibility that coassociation of p65, Stat3, and/or p21Cip1 plays a role in these findings, IP followed by Western blotting (WB) was performed in VSMCs. These experiments identified a p65/Stat3 complex and also showed that p65 and p21Cip1 coassociate in VSMCs (Figure 5D). We also detected reduced p65/p21Cip1 complex levels in Stat3Kd VSMCs, suggesting that Stat3 supports the p65/p21Cip1 interaction (Figure 5D).
We further investigated the relationship between Stat3 and p65/NF-κB, studying in detail their combinatorial binding at the putative NF-κB–binding sites in the Rantes promoter using quantitative ChIP with WT Co and Stat3Kd VSMCs. Tnf-α–stimulated Co VSMCs exhibited enhanced binding of both Stat3 and p65 at NF-κB–binding site no. 1 of the Rantes promoter (Figure 6, A and B). In contrast, Tnf-α–stimulated Stat3Kd VSMCs showed markedly attenuated p65 binding at NF-κB–binding site no. 1 of the Rantes promoter (Figure 6C), indicating that Stat3 is required for p65 binding at this site. We also observed enhanced Stat3 binding to NF-κB–binding site no. 2 following Tnf-α stimulation (Supplemental Figure 10A). While p65 binding was also enhanced at NF-κB–binding site no. 2 with Tnf-α stimulation, this was somewhat more modest than p65 binding at site no. 1 (Supplemental Figure 10B). Although not as robust as the data for site no. 1, Tnf-α–stimulated Stat3Kd VSMCs nonetheless displayed reduced p65 binding at NF-κB–binding site no. 2 of the Rantes promoter (Supplemental Figure 10C). Taken as a whole, these data indicate early p65 and Stat3 activation after arterial injury and show that the combined presence of these transcription factors, likely coassociated as a complex, is required for their effective binding to NF-κB–binding sites of the Rantes promoter in VSMCs.
Interdependent Stat3 and p65 binding to NF-κB–binding site no. 1 of the Rantes promoter. (A) ChIP of WT Co VSMCs with IP using anti-Stat3 antibody showing Stat3 binding to NF-κB–binding site no. 1 of the Rantes promoter without (Co) or with Tnf-α stimulation for 1, 2, 4, or 8 hours immediately prior to protein-DNA cross-linking (Co versus 2 hours and Co versus 4 hours, **P < 0.01; Co versus 8 hours, ***P < 0.005; n = 3 for all groups). (B) ChIP of WT Co VSMCs with IP using anti-p65 antibody showing p65 binding to NF-κB–binding site no. 1 of the Rantes promoter following Tnf-α stimulation (Co versus 1 hour, **P < 0.01; Co versus 2 hours, ****P < 0.001; Co versus 4 hours, ***P < 0.005; Co versus 8 hours, *P < 0.05; n = 3 for all groups). (C) ChIP of WT Stat3Kd VSMCs with IP using anti-p65 antibody showing p65 binding to NF-κB–binding site no. 1 of the Rantes promoter following Tnf-α stimulation (n = 3 for all groups). Data are shown as mean + SEM.
Tnf-α, but not Il-6, stimulates Rantes transcription in VSMCs. We investigated the upstream pathways leading to Rantes expression in VSMCs by evaluating the effect of treatment with Tnf-α versus Il-6, both potential activators of Stat3 and/or NF-κB. Tnf-α treatment led to a time-dependent increase in Rantes transcription, with 8 hours of Tnf-α exposure resulting in a greater than 450-fold increase in Rantes mRNA expression (Figure 7A). Surprisingly, Il-6 treatment for up to 8 hours (Figure 7B) or even 1 day (data not shown) did not appreciably alter Rantes mRNA levels. Given this, we compared Stat3 activation patterns in WT murine VSMCs and 3T3 fibroblasts. Il-6 treatment of VSMCs resulted in a gradual increase in p-Stat3. However, Tnf-α stimulation induced a rapid initial accumulation of p-Stat3 in VSMCs that waned with longer duration of Tnf-α treatment (Figure 7C). In contrast, Il-6 treatment of 3T3 cells caused a more robust increase in p-Stat3, but most notably, p-Stat3 was almost undetectable in 3T3 fibroblasts until after 8 hours of Tnf-α treatment (Figure 7C). Therefore, while Il-6 induces Stat3 phosphorylation, stimulation with Tnf-α leads to a differing pattern of Stat3 activation, with only Tnf-α able to induce Rantes expression in VSMCs.
Tnf-α, but not Il-6/gp130, stimulates Rantes transcription in VSMCs. (A) qRT-PCR for Rantes mRNA expression in WT VSMCs without (Co) or with Tnf-α stimulation for 1, 2, 4, or 8 hours (Co versus 1 hour, **P < 0.01; Co versus 2 hours, ***P < 0.005; Co versus 4 hours, *P < 0.05; Co versus 8 hours, ***P < 0.005; n = 3 for all groups). (B) qRT-PCR for Rantes mRNA expression in WT VSMCs without (Co) or with Il-6 stimulation for 1, 2, 4, or 8 hours (n = 3 for all groups). (C) WBs for p-Stat3 in WT VSMCs versus 3T3 cells without (Co) or with Tnf-α or Il-6 stimulation for 1, 2, 4, or 8 hours. Levels of Stat3 and β-actin are shown and were similar between groups. (D) WB for p-Stat3 in WT VSMCs pretreated with Tnf-α–R1–blocking antibody at the indicated concentrations and then stimulated with Tnf-α. Co lane: WB using IgG on VSMCs receiving Tnf-α stimulation but not Tnf-α–R1–blocking antibody. Levels of Stat3 and β-actin are shown and were similar between groups. (E) WT Co and gp130Kd VSMCs without (Co) or with Il-6 or Tnf-α treatment for 1, 2, 4, or 8 hours. No differences in Rantes mRNA expression were observed between cell types (n = 3 for all groups). Data are shown as mean + SEM.
We explored the involvement of the predominant Tnf-α receptor, Tnf-α receptor 1 (Tnf-α–R1), and gp130 (an Il-6 signal transducer) in these pathways. Using Tnf-α–R1–blocking antibody, we confirmed that Stat3 activation in response to Tnf-α was at least partially mediated via ligand binding at Tnf-α–R1 (Figure 7D). We next examined Rantes expression in VSMCs after knockdown of gp130 (gp130Kd) (Supplemental Figure 9D). Although the pattern of Rantes mRNA expression in gp130Kd VSMCs was consistent with our earlier data, we failed to detect any difference in the response to Tnf-α or Il-6 stimulation between Co and gp130Kd VSMCs (Figure 7E). These data indicate that Tnf-α–activated NF-κB/Stat3 signaling regulates Rantes transcriptional activation in VSMCs. Although the Il-6/Stat3 pathway may regulate Rantes in other cell types (17), our data suggest that Il-6/gp130 signaling has little effect on Rantes production in VSMCs.
Vascular Rantes expression is dependent on Tnf-α and Stat3 in vivo. Finally, we sought to confirm that a Tnf-α–initiated and Stat3-dependent pathway of acute Rantes production is operative in vivo. Thus, mice with genetic deletion of Tnf-α underwent arterial injury. Compared with vessels from WT mice, arteries from Tnfa–/– mice exhibited a significant reduction in Rantes mRNA expression at 6 hours after arterial injury (Figure 8A). Next, a conditional mouse line with inducible and specific Stat3 knockdown in smooth muscle cells (Stat3fl/fl;SM22α-Cre) was generated. Vascular specificity of SM22α-Cre for medial VSMCs was confirmed (see Methods), and although Stat3 knockdown was VSMC-specific and quantitative real-time PCR (qRT-PCR) was of entire femoral artery samples (including adventitia and other non-VSMC tissues), we observed more than 40% total vessel knockdown of Stat3 mRNA in induced Stat3fl/fl;SM22α-Cre mice (n = 8 for WT, n = 6 for Stat3fl/fl;SM22α-Cre; P = 0.05). Importantly, compared with vessels from WT mice, arteries from Stat3fl/fl;SM22α-Cre mice exhibited a significant reduction in Rantes mRNA expression at 6 hours after arterial injury (Figure 8B). These data validate our in vitro experiments and confirm that acute local vascular Rantes production is stimulated by Tnf-α and modulated by downstream NF-κB/Stat3 signaling.
Vascular Rantes expression is dependent on Tnf-α and Stat3 in vivo. (A) Rantes mRNA expression 6 hours after injury was decreased in femoral arteries from Tnfa–/– compared with WT mice (n = 5 for WT, n = 8 for Tnfa–/–; *P < 0.05). (B) Rantes mRNA expression 6 hours after injury was decreased in femoral arteries from Stat3fl/fl;SM22α-Cre compared with WT mice (n = 5 for WT, n = 6 for Stat3fl/fl;SM22α-Cre; *P < 0.05). Data are shown as mean + SEM.
Relatively little is known regarding the initiation of the vascular inflammatory program and to what extent VSMCs contribute to this process. We identified acute Rantes production by medial VSMCs following arterial injury. In VSMCs, stimulation by Tnf-α, but not Il-6, caused Stat3 activation and Rantes transcription — processes also under the higher-order control of p21Cip1. Stat3 and p65 coassociated in VSMCs, were individually obligatory for maximal Rantes expression, and were synergistic with respect to binding at NF-κB–binding domains of the Rantes promoter. Functionally, Tnf-α–initiated and Stat3-dependent VSMC Rantes production dictated T cell and macrophage recruitment during acute vascular remodeling, while local Rantes production modulated late neointimal formation.
This work was driven by our finding of marked early macrophage and T cell recruitment following arterial injury. The acute recruitment of these cells has not, to our knowledge, previously been characterized in detail following vascular injury. Nevertheless, the importance of T cells and macrophages during vascular wound repair is incontrovertible. Initial evidence arose from broad knockdown models, including clodronate-induced macrophage depletion (39), anti-CD11b antibody administration (8), and Rag–/– mice with absence of B and T lymphocytes (1), in which depletion of macrophages/lymphocytes/neutrophils led to reduced neointimal formation. While certain regulatory subtypes retard vascular inflammation (6, 7), the paradigm that macrophages and T cells generally enhance inflammation and neointimal formation has been reinforced by genetic deletion of key surface antigens such as P-selectin glycoprotein ligand-1 (12), CCR2 (10, 11), CXCR3 (5), and CX3CR1 (13) or the inhibition of specific chemokines including monocyte chemotactic protein-1 (Mcp-1) (11), stromal cell–derived factor-1 (Sdf-1) (2), and Rantes (14).
Rantes promoter activity (19, 36) and transcription (40) may be stimulated by Tnf-α and mediated by NF-κB in various non-VSMC populations. However, in mammary epithelial cells, it was recently proposed that Il-6 stimulation leads to Stat3 phosphorylation, increased concentrations of unphosphorylated Stat3, and eventually increased Rantes transcription (17). In rat-derived VSMCs, Il-6 is known to induce cell migration (41). While it is claimed that rat VSMC migration may be mediated by Il-6–induced Stat3 activation, supporting evidence has been inconsistent, including only a 2-fold increase in p-Stat3 levels following Il-6 VSMC stimulation (41) and putative Il-6 pathway (JAK2) inhibition causing only very modest attenuation of p-Stat3 levels (42). In direct opposition and suggesting a species-specific response, human VSMCs express only scant amounts of Il-6 receptor and are intrinsically unresponsive to Il-6 (43). Regardless of these controversies, our mouse models suggest Il-6/gp130 signaling does not regulate VSMC Rantes transcription but rather that this is Tnf-α mediated. This VSMC pathway of Tnf-α–stimulated Rantes production is reliant on both p65 and Stat3 signaling. Furthermore, we did not identify any classic Stat3-binding motifs within the Rantes promoter, thus reinforcing the role of Stat3 as a transcriptional cofactor involved with p65 binding at NF-κB–binding sites in this pathway. Adding complexity, although transcription complexes involving NF-κB and Stat3 in liver- and kidney-derived cells have been described, these complexes were inducible in response to Il-6 and/or Il-1 (16, 44). In contrast, our ChIP data suggest increased p65/Stat3 coassociation in response to Tnf-α. Therefore, based on our findings, we propose that stimulation of VSMCs by Tnf-α appears to lead to parallel but convergent activation of both the NF-κB and Stat3 signaling pathways, culminating in Rantes transcription. While the mechanisms of Tnf-α–mediated activation of NF-κB signaling are complex and beyond the scope of this discussion (45), in the case of VSMC Stat3 activation, we speculate that ligand binding to Tnf-α–R1, which itself is devoid of intrinsic tyrosine kinase activity, recruits constitutively active nonreceptor tyrosine kinases JAK2 and c-Src to the intracellular Tnf-α–R1 domain, culminating in Stat3 phosphorylation (46).
An interesting question raised by our work is why Tnf-α, rather than Il-6, is so dominant at achieving acute Stat3 activation and Rantes production in VSMCs. While we did not directly address this question experimentally, our data suggest that Tnf-α is at least partially responsible in vivo for stimulating acute Rantes production by VSMCs following arterial injury. This hypothesis is supported by the fact that local (including local vascular) Tnf-α levels are known to increase dramatically very early after an appropriate stimulus (47) — leading to the original classification of Tnf-α as an “immediate-early” gene (48). Our observation that acute Rantes production by VSMCs is governed by Tnf-α is consistent with an immediate-early local increase in Tnf-α following vascular injury, which may arise from several sources, including adherent monocytes (47) and platelets (49). Conversely, as compared with Tnf-α, Il-6 levels potentially fluctuate over a slower time course (43), with Il-6–dependent VSMC activation reliant on complex activation pathways involving exogenous soluble Il-6 receptor (43). Indeed, the fact that relevant Il-6/gp130 signaling pathways operate with slower kinetics than Tnf-α–related pathways, at least in VSMCs, was evidenced in our studies of Stat activation following VSMC stimulation with these cytokines (Figure 7C). Furthermore, Il-6 has been suggested to be of minimal importance during the acute vascular inflammatory response (50), and although controversial, evidence from Il6–/– mice indicates that Il-6 may play a protective role against atherosclerotic plaque progression (51). Therefore, our findings that Tnf-α (rather than Il-6) induces early Stat3 activation and VSMC Rantes production are consistent with our current conceptual understanding of the pathobiology of acute vascular injury and these signaling systems.
A theoretical criticism of our work is that possible contributions from platelet-derived Rantes were not considered. Indeed, platelet-derived Rantes and heteromers between Rantes and other chemokines may be deposited on endothelium, leading to mononuclear cell infiltration (14, 23, 52). However, although platelet contributions were not directly measured, the fact that T cell recruitment was dramatically attenuated with local but not BM depletion of Rantes strongly suggests that platelet contributions to vessel Rantes levels are functionally minimal in this clinically relevant arterial denudation model.
The acute production of Rantes by medial VSMCs is consistent with the fact that these cells also produce Mcp-1 within hours of vascular injury, with the time course of Mcp-1 production strikingly similar to that of Rantes (4). Consistent with simultaneous Mcp-1 and Rantes production by VSMCs is that, compared with WT to WT, WT to Rantes–/– mice exhibited only an approximately 60% reduction in macrophage recruitment (Figure 3B). Potentially, ongoing but attenuated macrophage recruitment in WT to Rantes–/– mice may be attributable to Mcp-1.
We validated our findings using p21–/– mice, an established model of increased inflammation and neointimal formation after vascular injury (2, 32, 33). These experiments verified a Tnf-α–stimulated NF-κB/Stat3/Rantes pathway of inflammatory cell recruitment and shed further light on the orchestration of acute events after arterial injury. While increased p21Cip1 expression has been reported 1 day after arterial injury (33), we identified an even greater increase in p21Cip1 at 6 hours after injury, which, based on this and other work (2), appears to limit VSMC cytokine production. Mechanistically, our data suggest that p21Cip1 regulates Rantes by restraining Stat3 transcription in VSMCs, a finding consistent with reports indicating p21Cip1 inhibits Stat3 activation (15). However, it is likely that p21Cip1 modulates Rantes via additional pathways. Direct p21Cip1 binding inhibits the activity of several transcription factors including Stat3 (15), c-Myc (53), and E2F (54), and as we show here, in VSMCs, p21Cip1 complexes with p65 in a Stat3-dependent manner (Figure 5D). Given that p21Cip1 and Stat3 also coassociate in VSMCs (2) and again bearing in mind our ChIP data, we speculate that p21Cip1 may form a ternary complex with p65 and Stat3, serving to inhibit the binding and/or transcriptional activity of this complex. Interestingly, the role of p21Cip1 in modulating Rantes transcription is distinct from its traditional role as a cell-cycle inhibitor (55). Therefore, while p21Cip1 controls cell-cycle progression and restrains VSMC proliferation (2), our data underscore the relatively novel paradigm that p21Cip1 and potentially other members of the cyclin-dependent kinase inhibitor family may additionally function as transcriptional cofactors, being able to both interact directly with DNA-binding proteins and modulate the activity of the coactivators and corepressors that associate with them (15, 56, 57).
Although not without controversy (58), it is generally accepted that VSMCs express CCR5 (59), a receptor for Rantes. However, CCR5 and CCR1, another Rantes receptor, are widely expressed on T cells, monocytes, and other inflammatory cells (58, 60). Adding complexity, both CCR5 and CCR1 also act as receptors for other ligands (27). While VSMCs may migrate in response to Rantes (22), the receptor or receptors responsible for this are unclear, as CCR1 or CCR5 antagonism does not affect VSMC migration or proliferation (31). In the vasculature, despite an initial contrary report (61), compared with Ccr5+/+Apoe–/– Cos, CCR5-deficient Apoe–/– mice appear to exhibit decreased atherosclerotic macrophage and T cell infiltration, decreased plaque area, reduced neointimal formation, and increased VSMC expression of Th2-associated Il-10, an antiinflammatory cytokine (30, 31). Paradoxically, genetic deletion of CCR1 in Apoe–/– mice may increase T cell infiltration and plaque deposition via enhanced production of proinflammatory and Th1-associated IFN-γ (30, 31). Nevertheless, systemic treatment with Met-Rantes, a Rantes receptor antagonist with affinity for CCR5 and CCR1 (27), led to reduced macrophage infiltration and decreased neointimal formation in wire-injured arteries of Apoe–/– mice (14). Likewise, in Ldlr–/– mice, systemic Met-Rantes administration reduced atherosclerotic plaque burden, increased plaque stability, and decreased T cell (83%) and macrophage (43%) infiltration (27) — results highly concordant with our experiments (Figure 3, A and B). These findings have also been broadly replicated using a novel Rantes antagonist [44AANA47]-Rantes (26). Furthermore, this latter study suggested that despite differences between the CCR5 and CCR1 response, antagonism of Rantes signaling is associated with reduced proinflammatory Th1 activity (26). Clinically, controversy exists regarding possible associations between serum RANTES levels and the presence of coronary artery disease (62, 63). However, individuals carrying a 32-bp CCR5 deletional mutation, CCR5Δ32, appear at reduced risk for cardiovascular disease (64). In summary, converging lines of evidence attest to the importance of Rantes signaling in vascular biology and strongly support the further study and clinical investigation of this pathway.
In conclusion, we examined acute events following arterial wire injury, identifying NF-κB/Stat3/Rantes signaling as a key factor dictating the early vascular inflammatory response program. Of relevance, murine arterial wire injury is analogous to clinical angioplasty and stenting; more than 1,300,000 inpatient angioplasty procedures were performed in 2006 in the United States alone (65). However, due to neointimal hyperplasia, a significant number of patients require repeat intervention. We are optimistic that novel insights into acute vascular injury, such as those presented here, will lead to improved and targeted therapies for the treatment of vascular diseases including atherosclerosis and other related inflammatory pathologies including arteritis, transplant vasculopathy, and pulmonary hypertension.
Mice. WT C57BL/6, Rantes–/–, and Tnfa–/– mice were obtained from Jackson Laboratories. p21–/– mice were provided by T. Jacks (Massachusetts Institute of Technology, Cambridge, Massachusetts, USA) (2). Stat3fl/fl;SM22α-Cre mice were derived by crossing SM22α-Cre mice (66) into Stat3fl/fl mice (67), producing mice with tamoxifen-inducible knockdown of Stat3 in tissues expressing SM22α (smooth muscle cells) at the time of tamoxifen treatment. Stat3fl/fl;SM22α-Cre mice were induced by intraperitoneal tamoxifen injection, 1 mg/d (in 0.1 ml volume) for 7 days, followed by a 1-week break, then a second cycle of 1.5 mg/d for 7 days. Specificity of SM22α-Cre for medial VSMCs was confirmed by crossing SM22α-Cre with R26R-EYFP mice (Jackson Laboratories), demonstrating that approximately 55% of medial VSMCs activate Cre and express YFP, with negligible YFP expression in other vascular tissues (data not shown). SM22α-Cre mice were provided by R. Feil (Technische Universität München, Munich, Germany), while Stat3fl/fl mice were provided by D. Levy (New York University, New York, New York, USA). Genotype was routinely confirmed by PCR of tail DNA using gene-specific probes. All experiments were approved by the National Heart, Lung, and Blood Institute Animal Care and Use Committee.
Bone marrow transplantation. BM was obtained from 8- to 12-week-old male WT and Rantes–/– mice after CO2 euthanasia. BM cell suspensions were flushed from femurs and tibias, filtered, and placed on ice. Recipient female mice were lethally irradiated with 9 Gy whole-body irradiation, with 5 × 106 unfractionated (male) BM cells then delivered by tail-vein injection. Successful engraftment was confirmed, prior to further experimentation, 10 weeks later by qRT-PCR for the presence or absence of Sry to distinguish female and male BM cells (primer sequences provided in Supplemental Methods).
Arterial wire injury, vessel fixation, and vessel harvest. Mice underwent femoral artery wire injury at 12–16 weeks of age or 20–24 weeks of age for BM transplanted mice, as previously described (2, 68), resulting in complete endothelial denudation. The surgeon was blinded to mouse genotype. For vessel harvesting, after humane euthanasia, the thorax was entered and the heart swiftly exposed. A generous rent in the right atrium was created. The left ventricle was punctured using a 20-gauge needle, and 20 ml of 1× PBS at 4°C was infused at approximately 2.5 ml/min. This procedure minimized intraluminal platelet and leukocyte content of harvested vessels, which may have confounded our results. Three methods of vessel harvesting were then used: (a) for PCR and VSMC outgrowth studies vessels were harvested directly, with no further manipulation other than dissection and removal. (b) For vessels intended for immunofluorescence staining, following PBS infusion, 20 ml of 1.5% paraformaldehyde plus 0.1% glutaraldehyde in 1× PBS at 4°C was infused at the same rate (69). Vessels were then harvested and placed in 20% sucrose in 1× PBS at 4°C overnight. The next day, vessels were embedded in OCT compound, prepared as fresh frozen slides (10-μm–thick sections), and stored at -80°C pending analysis. (c) For neointimal assessment, following PBS infusion, mice were perfused with 20 ml of 10% neutral buffered formalin at the same rate. Vessels were then harvested and placed in fresh 10% neutral buffered formalin overnight and transferred to 70% ethanol the following morning. Vessels were then embedded in paraffin, mounted on slides (5-μm–thick sections), and stained with H&E. Neointima was assessed as previously described (1, 2).
VSMCs. Cultured VSMCs were maintained in DMEM containing high glucose, l-glutamine, and sodium pyruvate (GIBCO 11995; Invitrogen) to which 10% FBS, 100 units/ml penicillin-streptomycin, and additional l-glutamine to a final concentration of 6 mM were added. This medium is henceforth referred to as complete DMEM. Primary VSMCs were obtained by outgrowth methods. In brief, aortas were harvested from 10- to 12-week-old WT and p21–/– mice. Aortas were minced and incubated in 1 mg/ml type 1A collagenase and 0.125 mg/ml elastase (C2674 and E0127 respectively; Sigma-Aldrich) in complete DMEM for 15 minutes at 37°C with gentle shaking. Tissue fragments were centrifuged, resuspended in complete DMEM, plated, and allowed to adhere. Cells were split after VSMC outgrowth occurred and maintained in complete DMEM. VSMCs used for all experiments were passage 6 to 10.
Tissue culture. VSMCs were plated at a density of 8.0 × 103 cells/cm2 for WT and 4.0 × 103 cells/cm2 for p21–/– to account for the greater rate of p21–/– VSMC proliferation (2). For Rantes and Stat3 expression and secretion experiments, WT and p21–/– VSMCs were grown to confluence. Medium was then aspirated, frozen at –80°C, and subsequently processed by Thermo Scientific Inc. using SearchLight chemiluminescence sandwich ELISA to quantitate Rantes protein secretion. VSMCs were also harvested at this time for qRT-PCR. VSMCs were counted by hemocytometer and protein data normalized to cell number.
For stimulation experiments, VSMCs and NIH/3T3 cells (CRL-1658; ATCC) were grown to confluence in complete DMEM and treated with murine Tnf-α or Il-6 (315-01A and 216-16 respectively; Peprotech), each at 50 ng/ml, for 1, 2, 4, or 8 hours. Cells were harvested and lysed in RIPA buffer for WB or harvested for RNA extraction and qRT-PCR. For Tnf-α–blocking experiments, confluent VSMCs were pretreated with Tnf-α–R1–blocking antibody (MAB430; R&D Systems) for 1 hour at the indicated concentrations. Cells were then stimulated for 1 hour with Tnf-α (50 ng/ml), after which cells were harvested for WB. For experiments involving shRNA-transduced cell lines, VSMCs were generally cultured as described above, but with the addition of 3 μg/ml puromycin to the culture medium.
Luciferase reporter assay. A pGL2 basic firefly luciferase vector containing the murine Rantes promoter sequence from –979 to +8 was donated by X. Ma (Cornell University, Ithaca, New York, USA) (70). Online promoter analysis using TFSEARCH v1.3 (http://www.cbrc.jp/research/db/TFSEARCH.html) identified 2 putative NF-κB–binding sites. These sites were mutated using the QuikChange Site-Directed Mutagenesis Kit (Stratagene) with mutation efficacy confirmed using DNA sequencing. Nonmutated, mutated, or pGL2 basic Co plasmids (Promega) were transfected into WT or p21–/– VSMCs using the Basic Nucleofector Kit for Primary Smooth Muscle Cells (Amaxa). VSMCs were also transfected with pRL-SV40 Renilla luciferase vector (Promega) as an internal Co. Each cell group was plated onto culture dishes and harvested after 48 hours, at confluency. Promoter activity was assessed using the Promega Dual-Luciferase Reporter Assay System. Luminescence was measured using a PerkinElmer MicroBeta 1450 JET luminometer.
shRNA knockdown. Stat3, p65, and gp130 were knocked down using Expression Arrest lentiviral shRNA from Open Biosystems. HEK293T cells (Open Biosystems) were transfected with lentiviral shRNA against Stat3 (RMM3981-97059843, clone ID TRCN0000071456), p65 (RMM3981-9622545, clone ID TRCN0000055346), gp130 (RMM3981-97053778, clone ID TRCN0000065391), or GFP (RHS4459). VSMCs were plated and infected with lentiviral shRNA after 24 hours while subconfluent. Six days after transduction, medium was replaced with complete DMEM containing 3 μg/ml puromycin to select for successful transduction, with cells maintained in this medium from this point forward. Knockdown efficacy was assessed by qRT-PCR and WB.
qRT-PCR. RNA was extracted from cultured VSMCs using the RNeasy Mini Kit (Qiagen), while RNA from vessels was extracted by pulverizing femoral artery sections with a motorized pestle in TRIzol Reagent (Invitrogen) according to the manufacturer’s instructions. RNA was reverse transcribed using 1 μg total RNA by annealing to random primers at 48°C in 100 μl total reaction volume using TaqMan Reverse Transcription Reagents (N8080234; Applied Biosystems). RNA expression levels were analyzed by qRT-PCR using iQ SYBR Green Supermix (Bio-Rad). A 2 μl volume from each cDNA synthesis (cDNA from 20 ng of total RNA) and primers at a final concentration of 0.625 μM were combined in a 20-μl reaction volume (primer sequences provided in Supplemental Methods). qRT-PCR was performed on an MJ Research Dyad Disciple thermal cycler with Chromo 4 fluorescence detector (Bio-Rad) by denaturation at 95°C for 10 minutes, followed by 40 amplification cycles as follows: 10 seconds at 95°C, 20 seconds at 57°C, and 30 seconds at 72°C. Data were analyzed using Bio-Rad MJOpticon Monitor v3.1 software. qRT-PCR results were confirmed by melting temperature analysis, with cDNA product size verified by electrophoresis on 1.25% agarose gels. cDNA sample quantifications were normalized to 18S RNA expression.
Immunofluorescence staining. Immunofluorescence staining was performed on fresh frozen slides with primary antibodies against p65 (ab7970; Abcam), Stat3 (4904; Cell Signaling Technologies), and (Tyr705) p-Stat3 (9131; Cell Signaling Technologies), all at 1:50 dilution, and against Rantes (MAB478, R&D Systems), CD115 (14-1152; eBioscience), and CD3 (ab5690; Abcam) at 1:100 dilution. Co slides were routinely stained in parallel by substituting the primary antibody for IgG or specific IgG isotypes from the same species and at the same final concentration as the primary antibody. Secondary antibodies were donkey anti-rat or -rabbit Alexa Fluor 488 (A-21208 and A-21206, respectively; Invitrogen) at 1:500 dilution or donkey anti-rat or -rabbit Rhodamine Red-X (712-295-150 and 711-295-152, respectively; Jackson ImmunoResearch Laboratories) at 1:200 dilution. Mounting medium containing DAPI (H-1200; Vector Laboratories) was then applied. Images were acquired using a Zeiss Axioskop plus light microscope with AxioVision V4.3 software, or a Zeiss LSM 510 UV laser scanning confocal microscope system (Carl Zeiss GmbH). All immunofluorescence staining was performed at least 8 times and using sections obtained from differing vessels/mice. Cell counting was performed by a blinded member of our laboratory with extensive experience in cell morphology and the techniques described above.
WBs. Bradford assay was used to determine protein concentration, and 50 μg of total protein was loaded into each sample well. Antibodies against p21Cip1 (556431; BD Biosciences — Pharmingen), p-Stat3 (9145; Cell Signaling Technologies), Stat3 (9139; Cell Signaling Technologies), or p65 (ab7090; Abcam) were used at 1:1000 dilution. Antibody against β-actin (A3854; Sigma-Aldrich) was used at 1:200,000 dilution. For IP, cells were lysed in NP40 buffer (75 mM NaCl, 1.0% NP40, 50 mM Tris [pH 8.0], protease inhibitors), and 200 μg of cell lysate was incubated with the indicated antibodies and/or isotype Co IgG and analyzed by WB.
Quantitative chromatin IP. Formalin cross-linked protein-DNA complexes in cell and tissue lysates were sonicated to an average size of approximately 500 bp. Complexes were precleared and IP using protein A sepharose beads (Invitrogen) and antibodies against Stat3 (sc-482; Santa Cruz Biotechnology Inc.), p65 (ab7970; Abcam), or isotype Cos. Subsequently, cross-linking was reversed by overnight incubation at 65°C and proteinase K treatment. Enriched specific promoter fragments were measured by qRT-PCR (primer sequences provided in Supplemental Methods). Relative Stat3 and p65 promoter occupancy were adjusted to the background content of the unrelated β-actin promoter sequence, isotype IgG Cos, and the initial sonicated chromatin input.
Statistics. For cell culture, each individual experiment was repeated at least 3 times. Experimental data were analyzed by unpaired 2-tailed Student’s t test or ANOVA followed by Neuman-Keuls multiple comparison test. Results are expressed as mean ± SEM. Differences were deemed significant at P < 0.05. Statistical analyses were performed using Prism, version 4.00 (GraphPad Software).
We thank T. Jacks for providing p21–/– mice, R. Feil for SM22α-Cre mice, and D. Levy for Stat3fl/fl mice. We also thank X. Ma for sharing reagents. We thank the staff of the Laboratory of Animal Medicine and Surgery facility and Robin Schwartzbeck for assistance with the transgenic mice. We also acknowledge the professional skills and advice of Christian A. Combs and Daniela Malide (Light Microscopy Core Facility, National Heart, Lung and Blood Institute, NIH), J. Philip McCoy (Flow Cytometry Core Facility, National Heart, Lung and Blood Institute, NIH), and Michelle Olive (Genome Technology Branch, National Human Genome Research Institute). This project was funded by the intramural research program of the National Heart, Lung and Blood Institute. R. Gupta and A. Lee were supported by the Howard Hughes Medical Institute–NIH Research Scholars Program. F. Fang is supported by the Chinese Embassy of Washington, DC, and The Central South University, Changsha, China.
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