Mediators of Inflammation
Volume 2017 (2017), Article ID 2401027, 12 pages
https://doi.org/10.1155/2017/2401027

Research Article

Stimulation of Alpha7 Nicotinic Acetylcholine Receptor Attenuates Nicotine-Induced Upregulation of MMP, MCP-1, and RANTES through Modulating ERK1/2/AP-1 Signaling Pathway in RAW264.7 and MOVAS Cells

Liping Liu,1,2 Hongxian Wu,¹ Qunan Cao,¹ Zhenzhen Guo,¹ Anmin Ren,¹ and Qiuyan Dai¹

¹Department of Cardiology, Shanghai General Hospital of Nanjing Medical University, Shanghai Jiaotong University, Shanghai, China
²Department of Cardiology, Yancheng First People’s Hospital, The Fourth Affiliated Hospital of Nantong Medical University, Jiangsu, China

Correspondence should be addressed to Qiuyan Dai; daiqiuyan@medmail.com.cn

Received 3 March 2017; Revised 4 September 2017; Accepted 27 September 2017; Published 16 November 2017

Academic Editor: Anshu Agrawal

Copyright © 2017 Liping Liu et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract.

Vagus nerve stimulation through alpha7 nicotine acetylcholine receptors (α7-nAChR) signaling had been demonstrated attenuation of inflammation. This study aimed to determine whether PNU-282987, a selective α7-nAChR agonist, affected activities of matrix metalloproteinase (MMP) and inflammatory cytokines in nicotine-treatment RAW264.7 and MOVAS cells and to assess the underlying molecular mechanisms. RAW264.7 and MOVAS cells were treated with nicotine at different concentrations (0, 1, 10, and 100 ng/ml) for 0–120 min. Nicotine markedly stimulated the phosphorylation of extracellular signal-regulated kinase1/2 (ERK1/2) and c-Jun in RAW264.7 cells. Pretreatment with U0126 significantly suppressed phosphorylation of ERK1/2 and further attenuated nicotine-induced activation of c-Jun and upregulation of MMP-2, MMP-9, monocyte chemotactic protein- (MCP-) 1, and regulated upon activation normal T cell expressed and secreted (RANTES). Similarly, nicotine treatment also increased phosphorylation of c-Jun and expressions of MMP-2, MMP-9, MCP-1, and RANTES in MOVAS cells. When cells were pretreated with PNU-282987, nicotine-induced activations of ERK1/2 and c-Jun in RAW264.7 cells and c-Jun in MOVAS cells were effectively inhibited. Furthermore, nicotine-induced secretions of MMP-2, MMP-9, MCP-1, and RANTES were remarkably downregulated. Treatment with α7-nAChR agonist inhibits nicotine-induced upregulation of MMP and inflammatory cytokines through modulating ERK1/2/AP-1 signaling in RAW264.7 cells and AP-1 in MOVAS cells, providing a new therapeutic for abdominal aortic aneurysm.

1. Introduction

Abdominal aortic aneurysm (AAA) is defined as a dilatation of abdominal aorta (almost exclusively infrarenal aorta) that reaches a diameter of 30 mm or more [1]. AAA often remains asymptomatic until it ruptures with a mortality rate of 80% [2]. Rather than a consequence of advanced atherosclerosis, AAA is a local representation of systemic vascular disease, with a differential molecular and cellular profile [3, 4]. AAA is characterized by dilatation of all layers of the arterial wall as a result of inflammatory infiltration, loss of elastin, and SMC apoptosis [3, 5]. Experimental data and studies of human AAA have identified that extensive inflammatory infiltrate in the media and adventitia is composed of macrophages and lymphocytes, which secret multiple cytokines, involving in the pathological process of AAA [6–8]. Matrix metalloproteinases (MMPs), derived from vascular smooth muscle cells (VSMCs) and macrophages, are secreted into the extracellular matrix and result in the destruction of elastin and weakening of the aortic wall [5].

Smoking is a very strong modifiable risk factor for AAA [9–13]. In a recent report of enrolling 18,782 participants aged ≥ 65 years in Southern Community Cohort Study (SCCS), over a median follow-up of 4.94 years, 40% of AAA were current smokers, and another 40% were former smokers [9]. Smoking, especially current smoking, significantly increased the risk of AAA (current: HR 5.55, 95% confidence interval (CI) 3.67 to 8.40; former: HR 1.91, 95% CI 1.27 to 2.87). Increased duration of smoking and daily cigarette quantity contribute to a higher risk of incident AAA, and the effects are dose dependent [11, 12]. Moreover, rates of AAA expansion and the risk of rupture are markedly elevated in those who continued to smoke. In a meta-analysis by Sweeting et al. [13], AAA growth rates were increased by about one-sixth and rupture rates were doubled in current smokers as compared to ex- or never smokers. Although prevalence, incidence, and mortality have declined because of a reduced smoking rate [14, 15], AAA remains the 16th leading cause of death in the USA among those aged above 65 years [9], thus highlighting the need for more efforts to improve the treatment and prognosis. Our previous study showed that c-Jun N-terminal kinase (JNK) inhibitor attenuated nicotine plus AngII-induced AAA formation by suppressing MMP-9, MMP2, monocyte chemotactic protein- (MCP-) 1, and regulated upon activation normal T cell expressed and secreted (RANTES) secretion from macrophages and VSMCs, suggesting that JNK was a signaling molecule in the pathogenesis of nicotine plus AngII-induced AAA [16]. However, distal signaling molecules or nuclear transcription factors involving in the signal transduction remain elusive.

Vagus nerve stimulation through alpha7 nicotine acetylcholine receptors (α7-nAChR) signaling, known as the cholinergic anti-inflammatory pathway, had been demonstrated attenuation of inflammation and improvement of inflammatory diseases, such as sepsis, pancreatitis, haemorrhagic shock and ischaemia/reperfusion, and postoperative ileus in experimental models [17]. Recent studies showed that vagus nerve stimulation may also have beneficial role in cardiovascular diseases through modulation of cytokine levels, which is dependent from heart rate variability [18]. Activation of α7-nAChR had been found to prevent the development and progression of AAA in CaCl₂ application mouse model in association with reduced inflammation and matrix degradation [19]. In the present study, we determined whether PNU-282987, a selective α7-nAChR agonist, affected activities of MMP-2 and MMP-9 and expressions of inflammatory cytokines MCP-1 and RANTES in nicotine treatment RAW264.7 and MOVAS cells.

2. Material and Methods

2.1. Reagents and Antibodies

Nicotine and PNU-282987 were obtained from Sigma-Aldrich. U0126 (a highly selective inhibitor of MEK1 and MEK2, which are kinase of ERK1/2) was from Cell Signaling Technology (CST). Monoclonal rabbit antiextracellular signal-regulated kinase1/2 (ERK1/2), antiphosphorylated ERK1/2, anti-c-Jun, antiphosphorylated c-Jun, antinuclear factor-κB (NF-κB) p65, and antiphosphorylated NF-κB p65 were from CST. Rat polyclonal antibody to MMP2, MCP-1, RANTES, and GAPDH were from Abcam. Mouse monoclonal anti-MMP9 and MMP2 were from Santa Cruz Biotechnology.

2.2. Cell Culture and Treatment

A mouse macrophage cell line (RAW264.7 cells) and mouse aortic smooth muscle cell (SMC) line (MOVAS cells) were bought from the American Type Culture Collection (Manassas, VA). Cells were cultured in high-glucose Dulbecco’s Modified Eagle Medium (DMEM, HyClone, Logan, UT, USA) supplemented with 10% fetal bovine serum (FBS, Gibco, Australia) at 37°C in a humidified, 5% CO₂ atmosphere. After starved in serum-free medium overnight, cells were treated with nicotine or PNU-282987. Additional experiments were performed with RAW264.7 cells pretreated with U0126 or PNU-282987 and MOVAS cells preincubated with PNU-282987 prior to exposing to nicotine.

2.3. Western Blot Analysis

Cells were washed twice with ice-cold phosphate-buffered saline (PBS), lysed with RIPA Lysis Buffer (Beyotime Institute of Biotechnology, Jiangsu, China), supplemented with phosphatase inhibitor (Sangon Biotechnology, Shanghai, China) and PMSF (Roche, Molecular Biochemicals, Mannheim, Germany), centrifuged, and quantified with a BCA protein assay kit (Beyotime Institute of Biotechnology, Jiangsu, China) according to the manufacturer’s instructions. Aliquots of total protein were separated by 10% sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-PAGE) and then transferred to polyvinylidene fluoride (PVDF) membranes (Bio-Rad Laboratories, Hercules, USA). Membranes were blocked in 5% nonfat milk/TBST (25 mM Tris-HCl, 150 mM NaCl, and 0.1% Tween-20; pH 7.4) for 1 h at room temperature and subsequently incubated with primary antibodies overnight at 4°C. After three washes, membranes were incubated with horseradish peroxidase- (HRP-) conjugated goat anti-rabbit or -mouse IgG for 1 h, washed again with TBST, and subsequently visualized using West-Pico ECL kit (Pierce, Rockford, USA).

2.4. Real-Time Reverse Transcription Polymerase Chain Reaction (RT-PCR)

Total RNA was extracted from RAW264.7 and MOVAS cells using TRIZOL reagent (Invitrogen, Carlsbad, USA) and reversely transcribed into cDNA with PrimeScript RT Master Mix (Takara, Kusatsu, Japan) according to the manufacturer’s protocol. Quantitative RT-PCR was performed using SYBR Premix Ex Taq (Takara, Kusatsu, Japan) on the Applied Biosystems ViiA™ 7 Real-Time PCR System. The specific primers used in the present study were as follows: MMP-9: 5′-GCCCTGGAACTCACACGACA-3′ (Forward) and 5′-TTGGAAACTCACACGCCAGAAG-3′ (Reverse); MMP-2: 5′-GATAACCTGGATGCCGTCGTG-3′ (Forward) and 5′-GGTGTGCAGCGATGAAGATGATA-3′ (Reverse); MCP-1: 5′-GCATCCACGTGTTGGCTCA-3′ (Forward) and 5′-CTCCAGCCTACTCATTGGGATCA-3′ (Reverse); RANTES 5′-GAAAGAACCGCCAAGTGTGT-3′ (Forward) and 5′-GCAAGCAGAAACAGGCAAAT-3′ (Reverse); and GAPDH: 5′-GTATGACTCTACCC ACGGCAAGT-3′ (Forward) and 5′-TTCCCGTTGATGACCAGCTT-3′ (Reverse). The cycle threshold (Ct) obtained for target gene expression was normalized to GAPDH, and the relative expression was calculated using the 2−ΔΔCt methods.

2.5. Statistical Analysis

Data were presented as mean ± standard deviations (SD). Densitometric analysis of protein bands in the Western blot was performed using ImageJ software from the National Institutes of Health. Data were analyzed by one-way ANOVA followed by the Dunnett’s test. Statistical analysis was conducted using SPSS version 22. was considered statistically significant.

3. Results

3.1. Nicotine Stimulated Phosphorylation of ERK1/2 and c-Jun in RAW264.7 Cells

Nicotine is the main ingredient of cigarette smoke, and plasma concentration of nicotine is rapidly increased after a single cigarette, ranging from 10–50 ng/ml [20]. To investigate the underlying mechanisms of nicotine-induced AAA, RAW264.7 cells were exposed to 10 ng/ml nicotine for 0, 10, 20, 30, 60, and 120 min. Western blot analysis (Figure 1(a)) revealed that 10 ng/ml nicotine resulted in significant increase in the phosphorylation of ERK1/2 and c-Jun from 10 min to 60 min; however, nicotine had no effect on p65 phosphorylation. Then, RAW264.7 cells were treated with nicotine for 30 min at the concentrations of 0, 1, 10, and 100 ng/ml. As seen in Figure 1(e), the phosphorylation of ERK1/2 and c-Jun was upregulated by nicotine, whereas the protein levels of p-p65 remained unchanged. These data suggest that nicotine may exert biological effects via modulating ERK1/2 and c-Jun signaling pathway in RAW264.7 cells.

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Figure 1: Nicotine stimulated the phosphorylation of extracellular signal-regulated kinase1/2 (ERK1/2) and c-Jun in RAW264.7 cells. (a) RAW264.7 cells were treated with 10 mg/ml nicotine for 0, 10, 20, 30, 60, and 120 min. (e) RAW264.7 cells were exposed to nicotine for 30 min at the concentrations of 0, 1, 10, and 100 mg/ml. Cell lysates were collected and protein levels of p-ERK1/2, ERK1/2, p-c-Jun, c-Jun, p-p65, and p65 were measured by Western blot. The band optical density values (means ± SD) of p-ERK1/2 (b, f), p-c-Jun (c, g), and p-p65 (d, h) were evaluated using ImageJ software, with all experiments being analyzed as three different independent experiments and GAPDH used as an internal control. and versus controls.

3.2. U0126 Abolished Nicotine-Induced Activations of ERK1/2 and c-Jun and Expression of MMP-9, MMP-2, MCP-1, and RANTES in RAW264.7 Cells

In order to further determine whether ERK1/2 and c-Jun signaling pathway is involved in nicotine-induced expression of MMP-9, MMP-2, MCP-1, and RANTES, RAW264.7 cells were pretreated with 10 μm and 20 μm U0126 for 30 min prior to 30 min or 3 h nicotine exposure at the concentration of 10 ng/ml. Nicotine-induced activation of ERK1/2 and c-Jun was significantly abolished by U0126 (Figure 2(a)). Also, nicotine-induced upregulation of MMP-9, MMP-2, MCP-1, and RANTES was remarkably decreased shown in Figure 2(d). Moreover, quantitative RT-PCR showed that U0126 inhibited nicotine-induced MMP-9, MMP-2, MCP-1, and RANTES mRNA expression (Figures 2(i), 2(j), 2(k), and 2(l)). The results indicate that nicotine induces upregulation of MMP-9, MMP-2, MCP-1, and RANTES through activating ERK1/2/c-Jun pathway in RAW264.7 cells.

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Figure 2: U0126 attenuated nicotine-induced activations of extracellular signal-regulated kinase1/2 (ERK1/2) and c-Jun and upregulation of matrix metalloproteinase- (MMP-) 9, MMP-2, monocyte chemotactic protein- (MCP-) 1, and regulated upon activation normal T cell expressed and secreted (RANTES) in RAW264.7 cells. (a) RAW264.7 cells were pretreated with 10 μm and 20 μm U0126 for 30 min prior to 10 ng/ml nicotine exposure for 30 min. (d) RAW264.7 cells were pretreated with 10 μm and 20 μm U0126 for 30 min prior to 10 ng/ml nicotine exposure for 3 h. (b, c, e–h) The intensity of protein bands (means ± SD) in the Western blot were quantified by using ImageJ software and normalized to GAPDH. Representative results from three independent experiments are shown. (i) MMP-9, (j) MMP-2, (k) MCP-1, and (l) RANTES mRNA levels were determined by real-time reverse transcription polymerase chain reaction. All experiments were analyzed as triplicate independent experiments. and versus controls; # and ## versus the group treated with nicotine.

3.3. Nicotine Increased Phosphorylation of c-Jun in MOVAS Cells

We also explored whether nicotine had any effect on the ERK1/2, c-Jun, and p65 in MOVAS cells. Similarly, MOVAS cells were treated with 10 ng/ml nicotine for 0, 10, 20, 30, 60, and 120 min. As shown in Figure 3(a), nicotine-induced phosphorylation of c-Jun markedly increased at 10 min and 20 min and then gone down from 30 min to 120 min. In contrast, nicotine suppressed ERK1/2 phosphorylation and had no effect on the activation of p65. Then, MOVAS cells were exposed to nicotine at various concentrations (0, 1, 10, and 100 ng/ml) for 30 min. The phosphorylation of c-Jun was significantly elevated at all three concentrations, whereas ERK1/2 phosphorylation was inhibited (Figure 3(e)). The activation of p65 was not affected by nicotine at different concentration. These data reveal that c-Jun may be an important transcription factor involving in nicotine-induced biological effects in MOVAS cells. Inconsistent with RAW264.7 cells, MOVAS cells treated with nicotine exhibited contrary tendency between ERK1/2 and c-Jun. It is worth mentioning that Cho et al. had showed that U0126 had no effect on TNFα-induced activation of c-Jun in VSMCs [21]. Therefore, we hypothesized that nicotine evoked different signal transduction pathway to play biological roles in different cell types.

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Figure 3: Nicotine increased the phosphorylation of c-Jun in MOVAS cells. (a) MOVAS cells were exposed to 10 ng/ml nicotine for 0, 10, 20, 30, 60, and 120 min. (e) MOVAS cells were treated with nicotine for 30 min at the concentrations of 0, 1, 10, and 100 ng/ml. The expression of phosphorylated extracellular signal-regulated kinase1/2 (p-ERK1/2), ERK1/2, p-c-Jun, c-Jun, p-p65, and p65 were analyzed with Western blot. (b–d, f–h) Densitometric analysis of protein bands was performed via ImageJ software. GAPDH was utilized as an internal control, and all experiments were analyzed as three different independent experiments. and versus controls.

3.4. PNU-282987 Suppressed Nicotine-Stimulated Activation of ERK1/2 and c-Jun and Upregulation of MMP-9, MMP-2, MCP-1, and RANTES in RAW264.7 Cells

The cholinergic anti-inflammatory pathway is composed of the efferent vagus nerve, the neurotransmitter acetylcholine, and α7-nAChR [17]. Recently, the potential role vagus nerve stimulation in cardiovascular disease has emerged [18]. To determine the effect of α7-nAChR on nicotine-stimulated expression of MMPs and inflammation cytokines, cells were stimulated in the presence of the α7-nAChR selective agonist. In the first experiment, RAW 264.7 cells were exposed to 10 μm PNU-282987 for 0, 15, 30, 60, 90, and 120 min. Western blot analysis showed that PNU-282987 markedly suppressed the phosphorylation of ERK1/2 and c-Jun (Figure 4(a)). Nevertheless, p65 phosphorylation had a descending tendency without statistical significance. Then, RAW264.7 cells were pretreated with PNU-282987 at various concentrations (0, 1, 10, and 100 μm) for 30 min prior to 10 ng/ml nicotine exposure for 30 min or 3 h. As shown in Figure 4(e), nicotine-induced activation of ERK1/2 and c-Jun was abolished by PNU-282987 at the concentrations of 10 and100 μm. At the same concentrations, PNU-282987 suppressed nicotine-stimulated upregulation of MMP-9, MMP-2, MCP-1, and RANTES (Figure 5(a)). In addition, quantitative RT-PCR showed that PNU-282987 also attenuated nicotine-induced MMP-9, MMP-2, MCP-1, and RANTES mRNA expression (Figures 5(f), 5(g), 5(h), and 5(i)). These results suggest that α7-nAChR agonist inhibits nicotine-induced upregulation of MMP-9, MMP-2, MCP-1, and RANTES through modulating ERK1/2/c-Jun signaling in RAW264.7 cells.

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Figure 4: PNU-282987 suppressed nicotine-stimulated activation of extracellular signal-regulated kinase1/2 (ERK1/2) and c-Jun in RAW264.7 cells. (a) RAW264.7 cells were treated with 10 μm PNU-282987 for 0, 15, 30, 60, 90, and 120 min. (e) RAW264.7 cells were pretreated with 10 μm PNU-282987 for 60 min prior to 10 ng/ml nicotine exposure for 30 min. Protein levels of p-ERK1/2, ERK1/2, p-c-Jun, c-Jun, p-p65, and p65 were measured by Western blot, and the intensity of protein bands (means ± SD) (b–d, f, g) were assessed using ImageJ software, with all experiments being analyzed as three different independent experiments and GAPDH used as an internal control. and versus controls; # and ## versus the group treated with nicotine.

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Figure 5: PNU-282987 abrogated nicotine-induced upregulation of matrix metalloproteinase- (MMP-) 9, MMP-2, monocyte chemotactic protein- (MCP-) 1, and regulated upon activation normal T cell expressed and secreted (RANTES) in RAW264.7 cells. (a) RAW264.7 cells were pretreated with 10 μm PNU-282987 for 60 min prior to 10 ng/ml nicotine exposure for 3 h. The band optical density values (means ± SD) of (b) MMP-9, (c) MMP-2, (d) MCP-1, and (e) RANTES in the Western blot were quantified by using ImageJ software and normalized to GAPDH. Representative results from three independent experiments are shown. (f) MMP-9, (g) MMP-2, (h) MCP-1, and (i) RANTES mRNA levels were examined by real-time reverse transcription polymerase chain reaction. All experiments were analyzed as triplicate independent experiments. and versus controls; # and ## versus the group treated with nicotine.

3.5. PNU-282987 Attenuated Nicotine-Induced Activations of c-Jun and Expression of MMP-9, MMP-2, MCP-1, and RANTES in MOVAS Cells

In the second experiment, MOVAS cells were treated with 10 μm PNU-282987 for 0, 15, 30, 60, 90, and 120 min. Western blot analyses indicated that ERK1/2 and c-Jun phosphorylation was remarkably decreased at different time points, whereas the phosphorylation of p65 was not changed (Figure 6(a)). Then, MOVAS cells were pretreated with PNU-282987 at various concentrations (0, 1, 10, and 100 μm) for 60 min prior to 10 ng/ml nicotine treatment for 30 min or 3 h. As shown in Figure 6(e), nicotine-induced activation of c-Jun was attenuated by PNU-282987 at the concentrations of 10 and 100 μm. The inhibition of ERK phosphorylation by nicotine was further enhanced in MOVAS cells pretreated with PNU-282987. Moreover, PNU-282987 suppressed nicotine-stimulated excretion of MMP-9, MMP-2, MCP-1, and RANTES from MOVAS cells (Figure 7(a)). Also, quantitative RT-PCR showed that PNU-282987 also reduced nicotine-induced mRNA expression of MMP-9, MMP-2, MCP-1, and RANTES shown in Figures 7(f), 7(g), 7(h), and 7(i). These results suggest that α7-nAChR agonist inhibits nicotine-induced expression of MMP-9, MMP-2, MCP-1, and RANTES via c-Jun in MOVAS cells.

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Figure 6: PNU-282987 inhibited nicotine-stimulated activation of c-Jun in MOVAS cells. (a) MOVAS cells were exposed to 10 μm PNU-282987 for 0, 15, 30, 60, 90, and 120 min. (e) MOVAS cells were pretreated with 10 μm PNU-282987 for 60 min prior to 10 ng/ml nicotine exposure for 30 min. Cell lysates were collected, and protein levels of phosphorylated extracellular signal-regulated kinase1/2 (p-ERK1/2), ERK1/2, p-c-Jun, c-Jun, p-p65, and p65 were measured by Western blot. (b–d, f, g) Densitometric analysis of protein bands was performed via ImageJ software, with all experiments being analyzed as three different independent experiments and GAPDH used as an internal control. and versus controls; # and ## versus the group treated with nicotine.

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Figure 7: PNU-282987 downregulated nicotine-induced expression of matrix metalloproteinase- (MMP-) 9, MMP-2, monocyte chemotactic protein- (MCP-) 1, and regulated upon activation normal T cell expressed and secreted (RANTES) in MOVAS cells. (a) MOVAS cells were pretreated with 10 μm PNU-282987 for 60 min prior to 10 ng/ml nicotine exposure for 3 h. The band optical density values (means ± SD) of (b) MMP-9, (c) MMP-2, (d) MCP-1, and (e) RANTES in the Western blot were quantified by using ImageJ software and normalized to GAPDH. Representative results from three independent experiments are shown. (f) MMP-9, (g) MMP-2, (h) MCP-1, and (i) RANTES mRNA levels were determined by real-time reverse transcription polymerase chain reaction. All experiments were analyzed as triplicate independent experiments. and versus controls; # and ## versus the group treated with nicotine.

4. Discussion

In the present study, we demonstrated for the first time that stimulation of α7-nAChR suppressed nicotine-induced upregulation of inflammatory cytokines and MMP. MCP-1 and RANTES, as representative of CC chemokine family, had also been demonstrated involvement in AAA development [7, 22] and thought to play greater roles than other chemokines [23]. MCP-1 promoted macrophage infiltration, increased the MMP-9 expression in SMCs, and induced apoptosis of SMCs within AAA, either through a direct mechanism or via activation of macrophages [22, 24, 25]. RANTES, similarly to MCP-1, acts on multiple immune cells and plays an important role in chronic and acute inflammation [26]. MMP-9 and MMP-2, which degrade the extracellular matrix, work in concert to form AAA, and both MMP-9 and MMP-2 knockout mice are resistant to aneurysm development [27]. Inflammation and extracellular matrix degradation play crucial roles in AAA formation. Therefore, it is likely that suppression of MCP-1, RANTES, MMP-9, and MMP-2 through activation of α7-nAChR resulted in the attenuation of nicotine-induced AAA development.

The molecular mechanisms associated α7-nAChR agonist with suppression of nicotine-induced AAA formation may be ERK1/2 and AP-1- (c-Jun-) mediated signaling pathway in macrophages and SMCs. ERK1/2 belongs to mammalian mitogen-activated protein kinase (MAPK) family, which play a crucial role in various cellular responses, including cell proliferation, differentiation, and survival [28, 29]. Transcription factor AP-1 family comprises multiple Jun (c-Jun, JunB, and JunD) and Fos (c-Fos, FosB, Fral, and Fra2) members [30]. AP-1 had been found involvement in several physiological and pathological cellular processes including proliferation, inflammation, differentiation, growth, apoptosis, cell migration, and transformation [30, 31]. This study showed that nicotine increased expression of MCP-1, RANTES, MMP-9, and MMP-2 through activating ERK1/2/AP-1 (c-Jun) signaling pathway in RAW264.7 cells and AP-1 (c-Jun) in MOVAS cells. These results indicated that AP-1 (c-Jun) might play an important role in nicotine-induced AAA formation, which is further confirmed by the report that AP-1 (c-Jun) was remarkably elevated in human AAA [32]. Stimulation of α7-nAChR by PNU-282987 significantly inhibited nicotine-induced activation of ERK1/2 and AP-1 (c-Jun) in RAW264.7 and MOVAS cells and then suppressed nicotine-stimulated upregulation of MCP-1, RANTES, MMP-9, and MMP-2. Interestingly, nicotine might activate c-Jun through different signaling pathways in RAW264.7 and MOVAS cells. Our previous study demonstrated that nicotine activated and PNU-282987 inhibited JNK signaling in MOVAS cells, which could be another upstream pathway of c-Jun [33]. The elucidation of such signaling pathways will reveal novel molecular targets that may provide a new therapeutic strategy for AAA. It needed to mention that nicotine could not evoke the activation of NF-κB p65 in this study. Although it is well known that NF-κB regulates expression of multiple inflammatory cytokines, it may play little role in the process of nicotine-induced secretion of MCP-1 and RANTES.

The nAChRs are a family of ligand-gated ion channel receptors composed of 17 subunits α1–α10, β1–β4, γ, δ, and ε [34]. In addition to the central and peripheral nervous system, the nAChRs have been identified in vascular tissue and immune cells [34, 35]. The different subunit combinations result in functionally diverse nAChR subtypes that have different ligand affinity, cation permeability, and signaling [36, 37]. The involvement of nAChR in nicotine-induced expression of inflammatory cytokines and MMP and development of AAA remains unknown. Nevertheless, accumulating evidence points towards a protective role for α7-nAChR in inflammation-based cardiovascular diseases. Cheng et al. showed that α7-nAChR activation reduced the expression of TNFα and IL-6 and alleviated viral myocarditis [38]. Treatment with PNU-282987 inhibited ADP-induced platelet aggregation in human platelets, and hematopoietic α7-nAChR deficiency increased number of peritoneal leukocytes and expression of inflammatory mediators by both peritoneal leukocytes (TNFα and CRP) and the spleen (TNFα) [39], both thought to be important risk factors in atherosclerotic lesion development [40]. Stimulation of α7-nAChR by AR-R1779 attenuates atherogenesis in apolipoprotein E-deficient mice treated with AngII possibly through an anti-inflammatory effect and reduction of blood pressure and lipid levels [41].

In contrast to nicotine that activates multiple nAChRs subtypes, PNU-282987 is a selected agonist for α7-nAChR. Thus, we inferred that distinct effects of nicotine and PNU-282987 might be mediated by differential nAChR subtypes. In accordance with the assumption, a recent study by de Moura and McMahon showed that PNU-282987 failed to substitute for the nicotine discriminative stimulus in male C57BL/6J mice [42]. Another study showed that nicotine-induced catecholamine release from the adrenal glands was modulated by α3β4nAChR, but not by α7nAChR [43].

5. Conclusion

Taken together, α7-nAChR agonist inhibits nicotine-induced upregulation of inflammatory cytokines and MMP through modulating ERK1/2/AP-1 signaling in RAW264.7 cells and AP-1 in MOVAS cells. α7-nAChR agonist is expected to be a new therapeutic strategy for AAA. However, more studies, experimental and clinical ones, are necessary to gain further insights into the function and signaling of nAChRs and offer rational therapeutic strategies.

Conflicts of Interest

The authors have no specific funding in relation to this research and no conflicts of interest to disclose.

Acknowledgments

This work was supported by grants from the Natural Science Foundation of China (NSFC; no. 81370415 and no. 81670399).

References

R. Erbel, V. Aboyans, C. Boileau et al., “2014 ESC guidelines on the diagnosis and treatment of aortic diseases: document covering acute and chronic aortic diseases of the thoracic and abdominal aorta of the adult. The task force for the diagnosis and treatment of aortic diseases of the European Society of Cardiology (ESC),” European Heart Journal, vol. 35, no. 41, pp. 2873–2926, 2014.

P. S. Basnyat, A. H. Biffin, L. G. Moseley, A. R. Hedges, and M. H. Lewis, “Mortality from ruptured abdominal aortic aneurysm in Wales,” British Journal of Surgery, vol. 86, no. 6, pp. 765–770, 1999.

I. M. Nordon, R. J. Hinchliffe, I. M. Loftus, and M. M. Thompson, “Pathophysiology and epidemiology of abdominal aortic aneurysms,” Nature Reviews Cardiology, vol. 8, no. 2, pp. 92–102, 2010.

I. M. Nordon, R. J. Hinchliffe, P. J. Holt, I. M. Loftus, and M. M. Thompson, “Review of current theories for abdominal aortic aneurysm pathogenesis,” Vascular, vol. 17, no. 5, pp. 253–263, 2009.

G. Ailawadi, J. L. Eliason, and G. R. Upchurch, “Current concepts in the pathogenesis of abdominal aortic aneurysm,” Journal of Vascular Surgery, vol. 38, no. 3, pp. 584–588, 2003.

T. Freestone, R. J. Turner, A. Coady, D. J. Higman, R. M. Greenhalgh, and J. T. Powell, “Inflammation and matrix metalloproteinases in the enlarging abdominal aortic aneurysm,” Arteriosclerosis, Thrombosis, and Vascular Biology, vol. 15, pp. 1145–1151, 1995.

A. E. Koch, G. K. Haines, R. J. Rizzo et al., “Human abdominal aortic aneurysms: immunophenotypic analysis suggesting an immune-mediated response,” The American Journal of Pathology, vol. 137, no. 5, pp. 1199–1213, 1990.

R. K. Middleton, G. M. Lloyd, M. J. Bown, N. J. Cooper, N. J. London, and R. D. Sayers, “The pro-inflammatory and chemotactic cytokine microenvironment of the abdominal aortic aneurysm wall: a protein array study,” Journal of Vascular Surgery, vol. 45, no. 3, pp. 574–580, 2007.

E. Jahangir, L. Lipworth, T. L. Edwards et al., “Smoking, sex, risk factors and abdominal aortic aneurysms: a prospective study of 18 782 persons aged above 65 years in the Southern Community Cohort Study,” Journal of Epidemiology and Community Health, vol. 69, no. 5, pp. 481–488, 2015.

T. B. Wilmink, C. R. Quick, and N. E. Day, “The association between cigarette smoking and abdominal aortic aneurysms,” Journal of Vascular Surgery, vol. 30, no. 6, pp. 1099–1105, 1999.

K. C. Kent, R. M. Zwolak, N. N. Egorova et al., “Analysis of risk factors for abdominal aortic aneurysm in a cohort of more than 3 million individuals,” Journal of Vascular Surgery, vol. 52, no. 3, pp. 539–548, 2010.

S. H. Forsdahl, K. Singh, S. Solberg, and B. K. Jacobsen, “Risk factors for abdominal aortic aneurysms: a 7-year prospective study: the Tromso study, 1994-2001,” Circulation, vol. 119, no. 16, pp. 2202–2208, 2009.

M. J. Sweeting, S. G. Thompson, L. C. Brown, J. T. Powell, and collaborators R, “Meta-analysis of individual patient data to examine factors affecting growth and rupture of small abdominal aortic aneurysms,” British Journal of Surgery, vol. 99, no. 5, pp. 655–665, 2012.

S. Svensjo, M. Bjorck, M. Gurtelschmid, K. Djavani Gidlund, A. Hellberg, and A. Wanhainen, “Low prevalence of abdominal aortic aneurysm among 65-year-old Swedish men indicates a change in the epidemiology of the disease,” Circulation, vol. 124, no. 10, pp. 1118–1123, 2011.

F. A. Lederle, “The rise and fall of abdominal aortic aneurysm,” Circulation, vol. 124, no. 10, pp. 1097–1099, 2011.

Z.-Z. Guo, Q.-A. Cao, Z.-Z. Li et al., “SP600125 attenuates nicotine-related aortic aneurysm formation by inhibiting matrix metalloproteinase production and CC chemokine-mediated macrophage migration,” Mediators of Inflammation, vol. 2016, Article ID 9142425, 11 pages, 2016.

M. Rosas-Ballina and K. J. Tracey, “Cholinergic control of inflammation,” Journal of Internal Medicine, vol. 265, no. 6, pp. 663–679, 2009.

C. Leib, H. A. Katus, and Z. Kaya, “Cholinergic control of inflammation in cardiovascular diseases,” Trends in Cardiovascular Medicine, vol. 23, no. 2, pp. 46–51, 2013.

A. Watanabe, T. Ichiki, H. Kojima et al., “Suppression of abdominal aortic aneurysm formation by AR-R17779, an agonist for the α7 nicotinic acetylcholine receptor,” Atherosclerosis, vol. 244, pp. 113–120, 2016.

P. F. Isaac and M. J. Rand, “Cigarette smoking and plasma levels of nicotine,” Nature, vol. 236, no. 5345, pp. 308–310, 1972.

A. Cho, J. Graves, and M. A. Reidy, “Mitogen-activated protein kinases mediate matrix Metalloproteinase-9 expression in vascular smooth muscle cells,” Arteriosclerosis, Thrombosis, and Vascular Biology, vol. 20, no. 12, pp. 2527–2532, 2000.

C. W. Moehle, C. M. Bhamidipati, M. R. Alexander et al., “Bone marrow–derived MCP1 required for experimental aortic aneurysm formation and smooth muscle phenotypic modulation,” The Journal of Thoracic and Cardiovascular Surgery, vol. 142, no. 6, pp. 1567–1574, 2011.

J. S. Colonnello, K. A. Hance, M. L. Shames et al., “Transient exposure to elastase induces mouse aortic wall smooth muscle cell production of MCP-1 and RANTES during development of experimental aortic aneurysm,” Journal of Vascular Surgery, vol. 38, no. 1, pp. 138–146, 2003.

Q. Wang, J. Ren, S. Morgan, Z. Liu, C. Dou, and B. Liu, “Monocyte chemoattractant protein-1 (MCP-1) regulates macrophage cytotoxicity in abdominal aortic aneurysm,” PLoS One, vol. 9, no. 3, article e92053, 2014.

C. Q. Yang, W. Li, S. Q. Li et al., “MCP-1 stimulates MMP-9 expression via ERK 1/2 and p38 MAPK signaling pathways in human aortic smooth muscle cells,” Cellular Physiology and Biochemistry, vol. 34, no. 2, pp. 266–276, 2014.

P. Conti and M. DiGioacchino, “MCP-1 and RANTES are mediators of acute and chronic inflammation,” Allergy and Asthma Proceedings, vol. 22, no. 3, pp. 133–137, 2001.

G. M. Longo, W. Xiong, T. C. Greiner, Y. Zhao, N. Fiotti, and B. T. Baxter, “Matrix metalloproteinases 2 and 9 work in concert to produce aortic aneurysms,” Journal of Clinical Investigation, vol. 110, no. 5, pp. 625–632, 2002.

S. Torii, T. Yamamoto, Y. Tsuchiya, and E. Nishida, “ERK MAP kinase in G₁ cell cycle progression and cancer,” Cancer Science, vol. 97, no. 8, pp. 697–702, 2006.

L. Chang and M. Karin, “Mammalian MAP kinase signalling cascades,” Nature, vol. 410, no. 6824, pp. 37–40, 2001.

Y. Qiao, H. He, P. Jonsson, I. Sinha, C. Zhao, and K. Dahlman-Wright, “AP-1 is a key regulator of proinflammatory cytokine TNFα-mediated triple-negative breast cancer progression,” Journal of Biological Chemistry, vol. 291, no. 10, pp. 5068–5079, 2016.

E. Shaulian, “AP-1—the Jun proteins: oncogenes or tumor suppressors in disguise?” Cellular Signalling, vol. 22, no. 6, pp. 894–899, 2010.

H. Abdul-Hussien, R. Hanemaaijer, R. Kleemann, B. F. Verhaaren, J. H. van Bockel, and J. H. Lindeman, “The pathophysiology of abdominal aortic aneurysm growth: corresponding and discordant inflammatory and proteolytic processes in abdominal aortic and popliteal artery aneurysms,” Journal of Vascular Surgery, vol. 51, no. 6, pp. 1479–1487, 2010.

Z.-Z. Li, Z.-Z. Guo, Z. Zhang et al., “Nicotine-induced upregulation of VCAM-1, MMP-2, and MMP-9 through the α7-nAChR-JNK pathway in RAW264.7 and MOVAS cells,” Molecular and Cellular Biochemistry, vol. 399, no. 1-2, pp. 49–58, 2014.

J. Lee and J. P. Cooke, “The role of nicotine in the pathogenesis of atherosclerosis,” Atherosclerosis, vol. 215, no. 2, pp. 281–283, 2011.

N. Santanam, B. A. Thornhill, J. K. Lau et al., “Nicotinic acetylcholine receptor signaling in atherogenesis,” Atherosclerosis, vol. 225, no. 2, pp. 264–273, 2012.

J. P. Changeux, “The acetylcholine receptor: a model for allosteric membrane proteins,” Biochemical Society Transactions, vol. 23, no. 2, pp. 195–205, 1995.

B. M. Conti-Tronconi, K. E. McLane, M. A. Raftery, S. A. Grando, and M. P. Protti, “The nicotinic acetylcholine receptor: structure and autoimmune pathology,” Critical Reviews in Biochemistry and Molecular Biology, vol. 29, pp. 69–123, 2008.

Z. Cheng, G. Li-Sha, Z. Jing-Lin et al., “Protective role of the cholinergic anti-inflammatory pathway in a mouse model of viral myocarditis,” PLoS One, vol. 9, no. 11, article e112719, 2014.

S. Kooijman, I. Meurs, M. van der Stoep et al., “Hematopoietic α7 nicotinic acetylcholine receptor deficiency increases inflammation and platelet activation status, but does not aggravate atherosclerosis,” Journal of Thrombosis and Haemostasis, vol. 13, no. 1, pp. 126–135, 2015.

R. Ross, “Atherosclerosis – an inflammatory disease,” The New England Journal of Medicine, vol. 340, no. 2, pp. 115–126, 1999.

T. Hashimoto, T. Ichiki, A. Watanabe et al., “Stimulation of α7 nicotinic acetylcholine receptor by AR-R17779 suppresses atherosclerosis and aortic aneurysm formation in apolipoprotein E-deficient mice,” Vascular Pharmacology, vol. 61, no. 2-3, pp. 49–55, 2014.

F. B. de Moura and L. R. McMahon, “The contribution of α4β2 and non-α4β2 nicotinic acetylcholine receptors to the discriminative stimulus effects of nicotine and varenicline in mice,” Psychopharmacology, vol. 234, no. 5, pp. 781–792, 2016.

A. J. Grottick, R. Wyler, and G. A. Higgins, “The α₄β₂ agonist SIB 1765F, but not the α₇ agonist AR-R 17779, cross-sensitises to the psychostimulant effects of nicotine,” Psychopharmacology, vol. 150, no. 2, pp. 233–236, 2000.