Skip to main content

Advertisement

Nrf-2 signaling inhibits intracranial aneurysm formation and progression by modulating vascular smooth muscle cell phenotype and function

Article metrics

Abstract

Background

Oxidative stress and vascular smooth muscle cell (VSMC) phenotypic modulation influence intracranial aneurysm (IA) formation and progression. Oxidative stress plays an important role in phenotype switching, and nuclear factor erythroid 2-related factor 2 (Nrf-2) is one of the main antioxidant systems. Unfortunately, little is known about how Nrf-2 signaling influences VSMC phenotype switches during IA pathogenesis.

Methods

We examined the effect of Nrf-2 activation IA on formation and progression in an elastase-induced rat IA model. We also developed a hydrogen peroxide (H2O2)-induced VSMC oxidative damage model. Then, we analyzed VSMC phenotype changes in the setting of Nrf-2 activation or inhibition in vitro. The proliferation, migration ability, and apoptosis rate of VSMCs were tested. Lastly, we measured the expression levels of antioxidant enzymes and inflammatory cytokines downstream of Nrf-2.

Results

Nrf-2 activation suppressed IA formation and progression in vivo. We confirmed Nrf-2 nuclear translocation and a VSMC switch from the contractile to synthetic phenotype. Nrf-2 activation inhibited the proliferation, migratory ability, and apoptosis rate enhanced by H2O2. Quantitative real-time polymerase chain reaction (PCR) and western blot analysis revealed that Nrf-2 activation promoted antioxidant enzymes and VSMC-specific marker gene expressions but decreased pro-inflammatory cytokine levels.

Conclusion

These results suggest that Nrf-2 exerts protective effects against IA development by preventing VSMCs from changing to a synthetic phenotype.

Background

Intracranial aneurysms (IAs) are pathological dilations at main bifurcations of cerebral arteries and are the most common cause of subarachnoid hemorrhage. Nearly 3–5% of the adult population carries unruptured IA [1]. The mechanisms of IA development and rupture remain unclear. Many factors such as blood flow wall shear stress, inflammation, oxidative stress, and apoptosis are involved in IA etiology [2]. The abnormal hemodynamic changes that can lead to endothelial cell dysfunction are now considered to be the initiating factor [3]. Several inflammatory mediators are triggered and then release large amounts of inflammatory cytokines and oxidative factors. This can cause a number of pathological processes including disruption of internal elastic laminate, vascular smooth muscle cell (VSMC) phenotype modulation, and dysfunctional extracellular matrix (ECM) remodeling [2,3,4]. When vessel walls degenerate, intracranial arteries become too weak to resist the blood dynamic force, and pouch-like dilatations of cerebral arteries occur.

VSMCs are a major cell type in vessel walls that carry out various functions. There are two different types of VSMCs: contractile and synthetic. Markers of contractile phenotype include smooth muscle 22 alpha (SM22α), smooth muscle alpha actin (αSMA), SM myosin heavy chain (MHC), h1-calponin, and smoothelin [5]. In response to pathologic stimuli such as inflammation and oxidative stress, contractile phenotype VSMCs can convert to the synthetic type; this phenotype modulation is associated with deceased expression of contractile genes [6]. During these changes, VSMCs lose their ability to contract but contribute to recruitment of pro-inflammatory cells and remodeling of the vessel wall ECM [6]. Switching to synthetic type VSMCs is hypothesized to play an important role in several cardiovascular diseases [7].

Oxidative stress is a key contributor to IA formation and rupture [8]. Oxidative damage caused by reactive oxygen species (ROS) can injure vessel walls by generating unstable free radicals and recruiting pro-inflammatory cells [5]. ROS also play an essential role in inflammatory disorders and VSMC phenotype modulation [9]. Nuclear factor erythroid 2-related factor 2 (Nrf-2), which belongs to the CNC (cap ‘n’ collar) family of transcription factors, is one of the main endogenous antioxidant systems. In stress conditions, Nrf-2 translocates from the cytoplasm to the nucleus where it regulates the expression of antioxidant and anti-inflammatory genes [10]. However, little is known about the significance of Nrf-2 in IA pathophysiology. In the current study, we tested the hypothesis that activation of Nrf-2 signaling can inhibit IA progression by modulating VSMC phenotype and function.

Methods

Patients and tissue samples

The Institutional Review Board of the Huashan Hospital of Fudan University approved this study. Informed consent was obtained from all patients. IA and superficial temporal artery (STA) samples were obtained during surgery. All specimens were fixed in 10% formaldehyde and embedded in paraffin.

Rat IA model

All animal procedures were carried out according to the protocol of our Institutional Animal Care and Use Committee. The experimental protocol was reviewed and approved by the Ethics Committee of the Huashan Hospital affiliated with Fudan University in Shanghai, People’s Republic of China. Male adult Sprague Dawley rats (body weight 200–220 g; Jiesijie, China) were divided into two groups (n = 10). IAs were induced as described previously [11]. Briefly, the right common carotid artery of rats was ligated, and 10 μL of 10 U/mL elastase was stereotactically injected into the basal cisterns through a small burr hole made 1.2 mm rostral and 0.7 mm lateral to the right of the bregma. The rats were anesthetized with 3% isoflurane throughout the procedure. All rats were fed a hypertensive diet after the surgery, and one group was treated with the Nrf-2 agonist tert-butylhydroquinone (tBHQ, MedChemExpress, NJ, USA) 50 mg/kg/d by gavage. After 30 days, rats were perfused with phosphate-buffered saline (PBS) and 4% paraformaldehyde (PFA) under deep anesthesia, then infused with bromophenol blue solution. Aneurysms were defined as an outpouching of weakened vessel walls, the diameters of which were 150% greater than the patent artery. All samples were processed immediately as described above for human specimens.

Hematoxylin and eosin (HE) staining and immunohistochemistry

Tissues were cut into 5-μM sections and placed on polylysine-coated slides prior to routine HE staining. For immunohistochemical analysis, anti-Nrf-2 (ab28947, Abcam, Cambridge, UK) (ab28947, Abcam, Cambridge, UK) was used for primary antibodies, and 3,3′-diaminobenzidine (DAB) plus chromogen (Thermo Fisher Scientific, Waltham, MA) was used for substrate visualization, according to the manufacturers’ protocols.

Immunofluorescence staining

Five-micrometer-thick sections were incubated at 4 °C overnight with anti- SM22α (1:400 dilution) and anti-αSMA (1:200 dilution) (Abcam, Cambridge, UK). They were then incubated with appropriate fluorescence-labeled secondary antibodies (1:1000 dilution) for 2 h at room temperature. Nuclei were stained with DAPI (1:1000 dilution). All images were obtained with a fluorescence microscope (Leica Microsystems, Oberkochen, Germany).

Rat VSMC isolation and culture

Primary rats VSMCs were isolated and cultured using previously described methods [12]. After VSMCs migrated from tissue pieces in Dulbecco’s minimum essential medium (DMEM; Gibco, Grand Island, NY) supplemented with 20% fetal bovine serum (FBS; Gemini, West Sacramento, CA), they were collected and cultured in DMEM supplemented with 10% FBS, 100 U/mL penicillin, and 100 mg/mL streptomycin. Cells were grown in a humidified incubator (Thermo Fisher Scientific) at 37 °C in a 5% CO2 atmosphere, and VSMCs at passages 3 to 8 were used for all experiments. VSMCs were treated with hydrogen peroxide (H2O2, 0.5 mM) for 12 h to induce oxidative damage and pre-treated with tBHQ (20 μM/mL) for 24 h and Nrf-2 inhibitor ML385 (MedChemExpress, NJ, USA) (5 μM/mL) for 72 h [13] before stimulation with H2O2. VSMCs were harvested for mRNA and protein analyses and functional testing. Each experiment was performed at least three times with triplicate cultures.

Cell viability and proliferation assay

To choose appropriate concentrations of H2O2 and tBHQ, cell viability was evaluated by a Cell Counting Kit-8 (CCK-8, Dojindo Molecular Technologies, Gaithersburg, MD) according to the manufacturer’s instruction. Cells were seeded in 96-well plate with 5 × 103 cells/well and were cultured until 80% confluent. After treatment with different dosages of H2O2 (10, 1, 0.5, 0.2, 0.1 mM) for 12 h and tBHQ (1, 10, 20, 30, 40, 50 μM/mL) for 24 h, 10 μL of CCK-8 solution was added into the culture medium of each well, and then cells were incubated in humidified 95% air and 5% CO2 for 2 h at 37 °C. To evaluate the influence of Nrf-2 signaling on proliferation, cell proliferation tests were performed as mentioned above after treatment with tBHQ and ML 385. Absorbance was measured at 450 nm using a microplate reader (Bio-Tek, Winooski, VT).

Intracellular ROS measurement

To determine intracellular ROS levels, cells were seeded in 6-well plate (1 × 105 cells/well). After treatment as described above, DCFH-DA fluorescence probes (1:1000 dilution; Beyotime, Haimen, China) were loaded, and cells were incubated for 1 h at 37 °C. Then, VSMCs were washed three times with serum-free DMEM and suspended in PBS. The fluorescence intensity of DCF was measured at wavelengths of 488 nm (excitation) and 525 nm (emission) in a flow cytometer (Thermo Fisher Scientific, Waltham, MA).

Apoptosis analysis

The Dead Cell Apoptosis Kit with Annexin V Alexa & propidium iodide (PI) (Invitrogen, Carlsbad, CA) was employed to measure the apoptosis rate. Cells were treated as mentioned above, and agent-free culture was used as negative control. Next, VSMCs were harvested and washed twice with PBS. Cells were resuspended in 1× annexin-binding buffer and then stained with 5 μL of PI and FITC Annexin-V for 15 min at room temperature in the dark. After the incubation period, 400 μL 1× annexin-binding buffer was added, and stained cells were measured by flow cytometry, analyzing fluorescence emission at 530 nm and excitation at 488 nm.

Hoechst staining

For staining, cells were seeded in 24-well plates at 2 × 104 cells/well and cultured to 60–70%. After treatment, cells were fixed with fixation buffer for 10 min. After being washed three times with PBS, cells were incubated in 0.2 mL Hoechst (Beyotime) for 5 min and then washed three times with PBS. The images were captured using a fluorescence microscope (Leica) at wavelength of 350 nm (excitation) and 460 nm (emission). The count of positive cells was analyzed by ImageJ software (National Institutes of Health, Bethesda, MD).

Cell migration assay

For wound healing assays, cells were seeded into 24-well plates, treated as described above, and cultured until 90% confluence. After scratching by a 10-μL pipette tip, the wound width was photographed and measured by ImageJ at 0 and 24 h. For transwell assays, cells suspensions of 5 × 104 cells/mL were seeded in the upper chambers and incubated with Nrf-2 agonist or inhibitor. After treatment with H2O2 for 12 h, DMEM with 10% FBS was added to the bottom chambers to stimulate migration. Cells in the upper chambers were scraped after 24 h. Migrated cells were fixed with 4% PFA and stained in crystal violet. Numbers of migrated cells were assessed under light microscopy by counting six fields.

RNA isolation and quantitative real-time polymerase chain reaction (qRT-PCR) analysis

Total RNA was extracted by using TRIzol (Takara, Kusatsu, Japan) according to the manufacturer’s protocol. For qRT-PCR analysis, cDNA was synthesized using ABScript II cDNA First-Strand Synthesis Kit under to manufacturer instructions. mRNA expression was evaluated with SYBR green-based PCR reactions. The results were analyzed using the ΔΔCt method and expressed as ratio of the internal control, glyceraldehyde 3-phosphate dehydrogenase (GAPDH).

Cytokine and chemokine analysis

Cellular supernatants were collected (centrifuge at 1000 g for 5 min) after cells were treated as mentioned above. We choose interleukin 1 beta (IL-1b), IL-6, monocyte chemoattractant protein 1 (MCP-1), and tumor necrosis factor alpha (TNF-a). Cytokines were measured via a MILLIPLEX MAP Rat CVD Panel (Millipore, Billerica, MA).

Western blot analysis

The proteins were collected using RIPA lysis buffer. To determine the expression of nuclear transcription factor Nrf-2, nuclear and cytoplasmic proteins were extracted separately. Cell lysates were separated by sodium dodecyl sulfate-polyacrylamide gel electrophoresis and then transferred to polyvinylidene fluoride membranes. After membranes were blocked, proteins were detected with the following primary antibodies (Abcam, Cambridge, UK): anti-Nrf-2 (Ab137550), anti-NAD(P)H quinone dehydrogenase 1 (NQO-1) (ab28947), anti-SM22α (ab14106), and anti-αSMA (ab7817). The membranes were exposed to X-ray after being probed with enhanced chemiluminescence and visualized with an imaging system (Tanon, Shanghai, China). The results were calculated by ImageJ software.

Statistical analysis

Each experiment was performed at least three times with triplicate groups. Data are the means ± standard errors of the mean. All statistical analyses were performed using one-way analysis of variance in IBM SPSS statistics 23 (IBM Corp., Armonk, NY), and figures were generated in GraphPad Prism software version 7.0 (GraphPad Inc., San Diego, CA). p < 0.05 was considered significant.

Results

Nrf-2 signaling can inhibit IA formation and progression in a rat IA model

We first assessed the effect of Nrf-2 activation on IA formation and progression in a rat model. Figure 1B (a, b) HE staining show vessel wall weakness. Fig 1B shows the degradation of vessel wall and myointimal hyperplasia which are characteristics of unruptured intracranial aneurysm wall. Compared with normal cerebral artery, thinning of tunica media is more significant in the experimental group. Figure 1A (a) through (e) show normal cerebral arteries, aneurysmal arteries, an aneurysm, multiple aneurysms, and a ruptured aneurysm, respectively. The aneurysms are more likely to occur at major branching brain arteries. We found the rat aneurysms located at bifurcation of Willis’ circle and anterior circulation. There were seven and one aneurysms formed in the control (one middle cerebral artery, five anterior circulation, and one posterior circulation) and tBHQ (one anterior circulation) groups, respectively. These five types of arteries corresponded to different scores. The aneurysmal score of the tBHQ group was much lower than in the control group, suggesting that tBHQ can decrease the incidence of aneurysm and rate of rupture. There was a significant difference in aneurysm incidence between the control and tBHQ groups. The Nrf-2 agonist tBHQ significantly inhibited IA formation and progression in vivo.

Fig. 1
figure1

The effect of Nrf-2 activation on IA formation and progression. a Rate of aneurysm formation and rupture in the control and tBHQ treatment groups. (a) normal vessels, (b) aneurysmal artery (AA), (c) aneurysm (IA), (d) multiple aneurysms (MIA), (e) ruptured aneurysm (MIA), (f) quantitative analysis of (a) through (e) in the control and tBHQ treatment groups (N = intracranial aneurysms amounts under different condition). b (a) HE staining of normal cerebral artery (bar = 50 μM), (b) HE staining of IA (scale bar = 50 μM), (c) aneurysmal scores of the control and tBHQ treatment groups. Aneurysmal scores in the control group were much higher than that in the tBHQ group. (a) through (e). A corresponding to aneurysmal score of 1 to 5.*p < 0.05 compared with the control group

Downregulation and nuclear translocation of Nrf-2 in human IA specimens

DAB staining demonstrated decreased Nrf-2 expression in IAs compared with STAs. Furthermore, Nrf-2 expression overlapped with the nucleus position in IA, indicating that more Nrf-2 translocated into the nucleus in IAs than STAs (Fig. 2A).

Fig. 2
figure2

a Nrf-2 expression and localization in human STA (a, b) and IA (c, d). The decreased Nrf-2 expression and Nrf-2 nuclear translocation can be observed in magnified images (b, d) (scale bar = 10 μM). b Expression levels of VSMC-specific markers SM22α (red)/αSMA (green) and DAPI (blue) in human STA and IA (scale bar = 50 μM). The decline of VSMC-specific markers was detected in IA. c Representative pictures of the control and tBHQ groups for SM22α (red)/αSMA (green) and DAPI (blue) in immunofluorescence staining (scale bar = 50 μM). Photomicrographs show the increase of SM22α/αSMA in the tBHQ treatment group compared with the control. d Positive cells (cells with Nrf-2 translocation) numbers in A were analyzed (N = 3). Fluorescence intensity of specific VSMC markers in the STA/IA and control/tBHQ groups (N = 3). *p < 0.05 compared with the control group. STA, superficial temporal artery; IA, intracranial aneurysm; tBHQ, tert-butylhydroquinone

VSMCs switched to the synthetic phenotype in human IA tissues

Based on previous studies, we chose SM22α and αSMA as markers of contractile phenotype VSMCs and found that levels of both were decreased in the synthetic phenotype. In STA, high immunofluorescent signals of SM22α/αSMA were detected in VSMCs with normal cellular morphology (Fig. 2B). However, SM22α and αSMA signals obviously declined in VSMCs in aneurysm walls (Fig. 2B), suggesting that VSMCs in IA walls switched to the synthetic phenotype.

Nrf-2 agonist tBHQ can help VSMCs maintain a contractile phenotype

As mentioned above, the Nrf-2 activator tBHQ can reduce IA formation and inhibit progression in a rat IA model. SM22α and αSMA expression in aneurysms we developed in the control and tBHQ groups were analyzed. Aneurysms in the tBHQ group were smaller in diameter and had a thicker wall, a higher proportion of VSMCs, and greater SM22α/αSMA expression (Fig. 2C). The results indicated that tBHQ prevented VSMCs from decreasing in number and changing to the synthetic phenotype.

H2O2 caused oxidative damage in VSMCs

We initially intended to develop a VSMC oxidative damage model by incubation with H2O2 in vitro. ROS upregulation is known to cause oxidative damage. Cell viability was detected by CCK-8 assays, and intracellular ROS levels were by measured by flow cytometry. As shown in Fig. 3A (a) and Fig. 3B, H2O2 (0.5 mM) induced obvious intracellular ROS accumulation but had little influence on cell viability (p < 0.05). This concentration was therefore used in subsequent experiments.

Fig. 3
figure3

a Cell viability assays. (a) Viability changes of VSMCs treated with different concentrations of H2O2. Data are the means ± standard errors of the mean. *p < 0.05 compared with the control group. (b) Viability changes of VSMCs treated with different concentrations of tBHQ. Data are the means ± standard errors of the mean. *p < 0.05 compared with the control group. b Intracellular ROS in the control and H2O2 groups. Data are the means ± standard errors of the mean. *p < 0.05 compared with the control group. c Effect of Nrf-2 activator and inhibitor on H2O2 induced intracellular ROS levels. (a) control, (b) H2O2, (c) tBHQ, (d) ML 385. Data are the means ± standard errors of the mean. DCFH-DA lobe was used to measure levels of intracellular levels of ROS. *p < 0.05 compared with the control group; #p < 0.05 compared with the H2O2 group

Nrf-2 activator tBHQ and Nrf-2 inhibitor ML 385 decreased and increased cellular ROS levels caused by H2O2, respectively

To access the protective effect of tBHQ on H2O2-induced cytotoxicity, VSMCs were treated with different tBHQ concentrations. At 20 μM/mL, tBHQ did not affect VSMC survival rate (Fig. 3A (b), p < 0.05). ML 385 treatment was performed as described by Biswal et al. [13]. Figure  3C shows H2O2 (0.5 mM) increased ROS levels yielding a twofold higher fluorescence intensity compared with the control group, but this was significantly reduced by tBHQ (p < 0.05). In contrast, intracellular ROS in the ML 385 group increased threefold compared to the H2O2 treatment group (p < 0.05). These results suggest that activation or inhibition of Nrf-2 could affect intracellular oxidative status.

Nrf-2 inhibition contributed to VSMC proliferation and migration

Proliferation and migration abilities are different in the two distinct smooth muscle cell phenotypes [14]. Generally, synthetic VSMCs exhibit higher growth and migratory activity than contractile VSMCs [15]. We assessed cell viability after 12 h of H2O2 treatment with or without Nrf-2 activation. We found VSMCs oxidized by H2O2 exhibited higher proliferation ability, while tBHQ attenuated the H2O2-induced growth rate increase. Conversely, ML 385 pretreatment exacerbated this effect (Fig. 4A, p < 0.05). VSMC motility was analyzed by wound healing and transwell assays. The results (Fig. 4B and C) demonstrated that oxidative damage could enhance VSMC migration, and ML 385 treatment promoted migratory activity compared with the H2O2 group. A significant inhibition of migration was observed when VSMCs were incubated with tBHQ (p < 0.05). These results indicate that Nrf-2 could modulate VSMC proliferation and migration by regulating cellular oxidative stress.

Fig. 4
figure4

Nrf-2 signal pathway modulates VSMC functions and apoptosis rate. a Cell proliferation assays. Data are the means ± standard errors of the mean. *p < 0.05 compared with the control group; #p < 0.05 compared with the H2O2 group. b Wound healing assays, representative images of HUVEC migration in the control, H2O2, tBHQ, and ML 385 groups in the scratch assay (scale bar = 50 μM). Data are the means ± standard errors of the mean. *p < 0.05 compared with the control group; #p < 0.05 compared with the H2O2 group. c Transwell assays, representative images of invasive cells in the lower chamber stained with crystal violet (scale bar = 50 μM). (a) control, (b) H2O2, (c) tBHQ, (d) ML 385. Data are the means ± standard errors of the mean. *p < 0.05 compared with the control group; #p < 0.05 compared with the H2O2 group. d Apoptosis rates as measured by flow cytometry. The Dead Cell Apoptosis Kit with Annexin V Alexa & propidium iodide (PI) was used to measure the apoptosis rate. (a) control, (b) H2O2, (c) tBHQ, (d) ML 385. Data are the means ± standard errors of the mean. *p < 0.05 compared with the control group; #p < 0.05 compared with the H2O2 group. e Apoptosis rates analyzed by Hoechst staining. (a) control, (b) H2O2, (c) tBHQ, (d) ML 385. Data are the means ± standard errors of the mean. *p < 0.05 compared with the control group; #p < 0.05 compared with the H2O2 group

Effect of tBHQ and ML 385 on H2O2-induced vascular smooth muscle cells apoptosis

Oxidative stress leads to apoptosis. Hoechst staining and flow cytometry were performed to examine the apoptosis rate. As predicted, the VSMC apoptosis rate increased significantly after treatment with H2O2. Next, we detected the effect of Nrf-2 signaling on H2O2-induced VSMC apoptosis. Consistent with the effect of Nrf-2 on oxidative stress, tBHQ suppressed apoptosis, while ML 385 promoted apoptosis by inhibiting Nrf-2 (Fig. 4D and E, p < 0.05).

Nrf-2 activation improves VSMC-specific gene expression

Several studies have described how oxidative stress can induce VSMCs to switch from the contractile to synthetic type. However, the role of Nrf-2, which is one of the most important antioxidant molecules in phenotypic modulation, is still unclear. Thus, qRT-PCR and western blot were performed to investigate the effect of Nrf-2 on the expression of VSMC-specific markers. To investigate whether tBHQ activates Nrf-2 or ML 385 inhibits Nrf-2, we analyzed Nrf-2 levels in the cytoplasm and nucleus. As shown in Fig. 5D, cytoplasmic Nrf-2 decreased and nuclear Nrf-2 increased after tBHQ treatment (p < 0.05). Conversely, ML 385 inhibited Nrf-2 nuclear translocation (p < 0.05). SM22α and αSMA mRNA and protein levels decreased in H2O2-incubated VSMCs. The inhibition of SM22α and αSMA was largely diminished in VSMCs pretreated with tBHQ, which was consistent with tBHQ-induced Nrf-2 nuclear translocation, whereas the Nrf-2 inhibitor ML 385 further exacerbated the decrease in both markers (Fig. 5A (a–c), Fig. 5C, p < 0.05).

Fig. 5
figure5

Effects of Nrf-2 signaling on VSMC-specific markers, antioxidant enzymes, and inflammatory cytokines. Representative images of experiments performed in triplicate are presented. a Fold changes of Nrf-2, downstream antioxidant enzymes, and inflammatory cytokines mRNA levels. Data are the means ± standard errors of the mean. *p < 0.05 compared with the control group; #p < 0.05 compared with the H2O2 group. b Inflammatory cytokines analyzed by MILLIPLEX MAP Rat CVD Panel. Data are the means ± standard errors of the mean. *p < 0.05 compared with the control group; #p < 0.05 compared with the H2O2 group. c Western blot analysis of VSMC specific markers SM22α, and αSMA. Data are the means ± standard errors of the mean. *p < 0.05 compared with the control group; #p < 0.05 compared with the H2O2 group d Western blot analysis of Nrf-2 in the cytoplasm and nuclear fractions, antioxidant enzyme NQO-1, Data are the means ± standard errors of the mean. *p < 0.05 compared with the control group; #p < 0.05 compared with the H2O2 group  

Impact of Nrf-2 activation on oxidative redox balance and inflammation

Nrf-2 is an important endogenous antioxidant defense molecule. Many enzymes downstream of the Nrf-2 pathway are primary components of the antioxidant system, also known as phase II detoxifying enzymes. The antioxidant enzymes examined by qRT-PCR and western blot included NQO-1, glutamate-cysteine ligase catalytic subunit (GCLC), and superoxide dismutase 1 (SOD 1). Inflammatory cytokines and oxidative stress are closely related. qRT-PCR and MILLIPLEX MAP were performed to detect inflammatory cytokines including IL-1b, IL-6, MCP-1, and TNF-a. Figure 5A and B shows that tBHQ increased antioxidant enzyme gene expression and downregulated cytokine levels by activating Nrf-2 (p < 0.05). ML 385 aggravated oxidative damage by upregulating inflammatory cytokines and inhibited the transcription of genes encoding antioxidant enzymes (p < 0.05).

Discussion

The mechanism of IA development is still unclear. Many pathological factors like oxidative stress, inflammation, dysregulated hemodynamics, and extracellular matrix degeneration contribute to their formation and progression [16]. The interaction between oxidative stress and inflammation is a key mechanism of endothelial dysfunction and arterial damage. A role of VSMCs phenotype switching has been described in IAs, atherosclerosis, and aortic aneurysms. Oxidative stress can accelerate inflammation directly and indirectly, which further increases oxidative stress. This can induce phenotypically switched VSMCs to stimulate pro-inflammatory processes, extracellular matrix remodeling, and mural cells apoptosis, all of which eventually contribute to IA formation and rupture. Numerous lines of evidence indicate that VSMC phenotypic modulation is associated with IA formation, growth, and rupture [17,18,19].

Nrf-2, a basic leucine zipper transcription factor, plays a critical role in modulating cellular redox balance by promoting the transcription of detoxifying and antioxidant genes. Under oxidative conditions, Nrf-2 separates from Keap1 in the cytoplasm and translocates to the nucleus, which leads to the transcription of phase II detoxification enzymes and anti-inflammatory proteins. Researchers previously demonstrated that VSMCs phenotypes are influenced by inhibiting ROS generation, and this is important for maintaining vascular homeostasis [20]. Other findings also suggest that Nrf-2 could affect VSMC functions by reducing oxidative stress [21, 22]. We hypothesized that Nrf-2 pathway activation can prevent VSMCs from switching to the synthetic type by modulating oxidative stress and exerting protective effects against IA development.

We first examined the role of Nrf-2 pathway activation in vivo. An elastase-induced rat IA model was developed, and arteries were divided into five different types: normal cerebral arteries, aneurysmal arteries, aneurysms, multiple aneurysms, and ruptured aneurysms. After 30 days of treatment with Nrf-2 agonist tBHQ, there were lower aneurysmal scores and less IA formation and rupture compared with the control (Fig. 1). This indicates that Nrf-2 activation can suppress IA formation and progression. Consistent with our data, Zeng et al. reported that increased Nrf-2 levels help inhibit acute aortic dissection formation, which involves a pathological mechanism similar to IA [23]. In the presence of stimulating factors, Nrf-2 translocates into the nucleus and promotes downstream target genes expression by binding to the antioxidant response element. Our immunohistochemical results revealed stabilized Nrf-2 distributed in the cytoplasm of STAs, while downregulation and nuclear translocation were found in aneurysm walls (Fig. 2A). Nakajima et al. detected VSMCs phenotypic modulation in human aneurysmal walls and concluded that this process was related to aneurysm remodeling and rupture [24]. We found VSMC morphological changes, decreased SM22α/αSMA expression, and loss of mural VSMCs in IA, all of which are characteristic of IA walls (Fig. 2B). In the rat IA model, SM22α/αSMA was upregulated and aneurysm diameter was smaller after tBHQ treatment (Fig. 2C). These results suggest that Nrf-2 activation inhibits IA development by modulating VSMCs phenotype.

To investigate how Nrf-2 contributes to VSMC phenotypic switching, we examined the effect of Nrf-2 activation or inhibition on VSMC phenotype changes and functions in vitro. H2O2 can promote ROS generation, which is a central molecular component of oxidative stress and is widely used to induce cellular damage [25, 26]. We selected tBHQ as a Nrf-2 activator and ML 385 as Nrf-2 inhibitor, since they are well-studied and specific for Nrf-2 [13, 27, 28]. We observed that tBHQ decreased ROS generation while ML 385 promoted significant ROS accumulation (Fig. 3C). The results of cell proliferation and migration tests revealed that Nrf-2 activation exerts a negative effect on proliferative and migratory abilities. Two different methods confirmed that Nrf-2 activation decreased apoptosis (Fig. 4). Therefore, Nrf-2, which has regulatory roles in VSMC proliferation, migration, and apoptosis, is also associated with vascular remodeling that leads to IA formation and progression. We demonstrated that VSMCs switched to the synthetic phenotype after oxidative treatment, but while tBHQ helped, VSMCs maintain contractile phenotype according to qRT-PCR and western blot results. Conversely, ML 385 profoundly suppressed VSMC-specific marker expression (Fig. 5). The underlying mechanism may involve upregulation of antioxidant enzymes, decreased pro-inflammatory cytokine expression, and less intracellular ROS accumulation (Fig. 3, Fig. 5). When SM22α/αSMA levels are decreased, VSMCs develop increased capacities for proliferation, migration, and secretion of pro-remodeling factors and pro-inflammatory cytokines [29, 30]. VSMCs undergoing phenotypic switching can also aggravate oxidative stress and inflammation. These results are consistent with the functional changes described above and suggest that Nrf-2 modulates VSMC phenotype switches by affecting antioxidant and anti-inflammatory protein expression.

Conclusion

In summary, our results provide novel evidence that Nrf-2 signaling can inhibit IA formation and progression by regulating VSMC phenotypes. The Nrf-2 agonist tBHQ decreases the rates of IA formation and rupture and increases VSMC contractile gene expression by promoting Nrf-2 nuclear translocation (Fig. 6). The Nrf-2 antagonist ML 385 reverses this effect. Although prior studies have found a close relationship between VSMC phenotype switching and IA formation and rupture, none have assessed the role of the Nrf-2 signal pathway. Our findings provide a theoretical basis for research into novel pharmacologic therapies.

Fig. 6
figure6

Schematic illustrating how Nrf-2 activation regulates phenotypic modulation. Under oxidative-stimulating conditions, Nrf-2 is activated and translocates into the nucleus. Nrf-2 signal pathway activation promotes expression of VSMC-specific markers SM22α and αSMA. The underlying mechanism may be that Nrf-2 upregulates expression levels of its downstream antioxidant enzymes and inhibits pro-inflammatory cytokines

Availability of data and materials

Data generated and analyzed as part of this study are included in the manuscript or are available upon request from the corresponding author.

Abbreviations

ECM:

Extracellular matrix

HE:

Hematoxylin and eosin

IA:

Intracranial aneurysm

MHC:

Myosin heavy chain

NQO-1:

NAD(P)H quinone dehydrogenase 1

Nrf-2:

Nuclear factor erythroid 2-related factor 2

PCR:

Polymerase chain reaction

ROS:

Reactive oxygen species

SM22α:

Smooth muscle 22 alpha

SM-α-actin:

Smooth muscle alpha actin

tBHQ:

Tert-butylhydroquinone

VSMC:

Vascular smooth muscle cell

References

  1. 1.

    Etminan N, Rinkel GJ. Unruptured intracranial aneurysms: development, rupture and preventive management. Nat Rev Neurol. 2016;12(12):699–713. https://doi.org/10.1038/nrneurol.2016.150.

  2. 2.

    Chalouhi N, Hoh BL, Hasan D. Review of cerebral aneurysm formation, growth, and rupture. Stroke. 2013;44(12):3613–22. https://doi.org/10.1161/STROKEAHA.113.002390.

  3. 3.

    Signorelli F, Sela S, Gesualdo L, et al. Hemodynamic stress, inflammation, and intracranial aneurysm development and rupture: a systematic review. World Neurosurg. 2018;115:234–44. https://doi.org/10.1016/j.wneu.2018.04.143.

  4. 4.

    Liu P, Song Y, Zhou Y, et al. Cyclic mechanical stretch induced smooth muscle cell changes in cerebral aneurysm progress by reducing collagen type IV and collagen type VI levels. Cell Physiol Biochem. 2018;45(3):1051–60. https://doi.org/10.1159/000487347.

  5. 5.

    Starke RM, Chalouhi N, Ding D, et al. Vascular smooth muscle cells in cerebral aneurysm pathogenesis. Transl Stroke Res. 2014;5(3):338–46. https://doi.org/10.1007/s12975-013-0290-1.

  6. 6.

    Wang G, Jacquet L, Karamariti E, Xu Q. Origin and differentiation of vascular smooth muscle cells. J Physiol. 2015;593(14):3013–30. https://doi.org/10.1113/JP270033.

  7. 7.

    Wall VZ, Bornfeldt KE. Arterial smooth muscle. Arterioscler Thromb Vasc Biol. 2014;34(10):2175–9. https://doi.org/10.1161/ATVBAHA.114.304441.

  8. 8.

    Starke RM, Chalouhi N, Ali MS, et al. The role of oxidative stress in cerebral aneurysm formation and rupture. Curr Neurovasc Res. 2013;10(3):247–55.

  9. 9.

    Galougahi KK, Ashley EA, Ali ZA. Redox regulation of vascular remodeling. Cell Mol Life Sci. 2016;73(2):349–63. https://doi.org/10.1007/s00018-015-2068-y.

  10. 10.

    Keleku-Lukwete N, Suzuki M, Yamamoto M. An overview of the advantages of KEAP1-NRF2 system activation during inflammatory disease treatment. Antioxid Redox Signal. 2018;29(17):1746–55. https://doi.org/10.1089/ars.2017.7358.

  11. 11.

    Nuki Y, Tsou T-L, Kurihara C, Kanematsu M, Kanematsu Y, Hashimoto T. Elastase-induced intracranial aneurysms in hypertensive mice. Hypertens. 2009;54(6):1337–44. https://doi.org/10.1161/HYPERTENSIONAHA.109.138297.

  12. 12.

    Zhu Q, Ni X-Q, Lu W-W, et al. Intermedin reduces neointima formation by regulating vascular smooth muscle cell phenotype via cAMP/PKA pathway. Atherosclerosis. 2017;266:212–22. https://doi.org/10.1016/j.atherosclerosis.2017.10.011.

  13. 13.

    Singh A, Venkannagari S, Oh KH, et al. Small molecule inhibitor of NRF2 selectively intervenes therapeutic resistance in KEAP1-deficient NSCLC tumors. ACS Chem Biol. 2016;11(11):3214–25. https://doi.org/10.1021/acschembio.6b00651.

  14. 14.

    Davis-Dusenbery BN, Wu C, Hata A. Micromanaging vascular smooth muscle cell differentiation and phenotypic modulation. Arterioscler Thromb Vasc Biol. 2011;31(11):2370–7. https://doi.org/10.1161/ATVBAHA.111.226670.

  15. 15.

    Rensen SSM, Doevendans PAFM, van Eys GJJM. Regulation and characteristics of vascular smooth muscle cell phenotypic diversity. Neth Heart J. 2007;15(3):100–8.

  16. 16.

    Weir B. Unruptured aneurysms. J Neurosurg. 2002;97(5):1011–3. https://doi.org/10.3171/jns.2002.97.5.1011.

  17. 17.

    Sun L, Zhao M, Zhang J, et al. MiR-29b downregulation induces phenotypic modulation of vascular smooth muscle cells: implication for intracranial aneurysm formation and progression to rupture. Cell Physiol Biochem. 2017;41(2):510–8. https://doi.org/10.1159/000456887.

  18. 18.

    Frosen J, Piippo A, Paetau A, et al. Remodeling of saccular cerebral artery aneurysm wall is associated with rupture: histological analysis of 24 unruptured and 42 ruptured cases. Stroke. 2004;35(10):2287–93. https://doi.org/10.1161/01.STR.0000140636.30204.da.

  19. 19.

    Chalouhi N, Ali MS, Jabbour PM, et al. Biology of intracranial aneurysms: role of inflammation. J Cereb Blood Flow Metab. 2012;32(9):1659–76. https://doi.org/10.1038/jcbfm.2012.84.

  20. 20.

    Zhong L, He X, Si X, et al. SM22alpha (smooth muscle 22alpha) prevents aortic aneurysm formation by inhibiting smooth muscle cell phenotypic switching through suppressing reactive oxygen species/NF-kappaB (nuclear factor-kappaB). Arterioscler Thromb Vasc Biol. 2019;39(1):e10–25. https://doi.org/10.1161/ATVBAHA.118.311917.

  21. 21.

    Levonen A-L, Inkala M, Heikura T, et al. Nrf2 gene transfer induces antioxidant enzymes and suppresses smooth muscle cell growth in vitro and reduces oxidative stress in rabbit aorta in vivo. Arterioscler Thromb Vasc Biol. 2007;27(4):741–7. https://doi.org/10.1161/01.ATV.0000258868.80079.4d.

  22. 22.

    Ashino T, Yamamoto M, Yoshida T, Numazawa S. Redox-sensitive transcription factor Nrf2 regulates vascular smooth muscle cell migration and neointimal hyperplasia. Arterioscler Thromb Vasc Biol. 2013;33(4):760–8. https://doi.org/10.1161/ATVBAHA.112.300614.

  23. 23.

    Liu W, Wang B, Wang T, et al. Ursodeoxycholic acid attenuates acute aortic dissection formation in angiotensin II-infused apolipoprotein E-deficient mice associated with reduced ROS and increased Nrf2 levels. Cell Physiol Biochem. 2016;38(4):1391–405. https://doi.org/10.1159/000443082.

  24. 24.

    Nakajima N, Nagahiro S, Sano T, Satomi J, Satoh K. Phenotypic modulation of smooth muscle cells in human cerebral aneurysmal walls. Acta Neuropathol. 2000;100(5):475–80.

  25. 25.

    Arcanjo NO, Andrade MJ, Padilla P, Rodriguez A, Madruga MS, Estevez M. Resveratrol protects lactobacillus reuteri against H2O2- induced oxidative stress and stimulates antioxidant defenses through upregulation of the dhaT gene. Free Radic Biol Med. 2019;135:38–45. https://doi.org/10.1016/j.freeradbiomed.2019.02.023.

  26. 26.

    Lee J, Song K, Huh E, Oh MS, Kim YS. Neuroprotection against 6-OHDA toxicity in PC12 cells and mice through the Nrf2 pathway by a sesquiterpenoid from Tussilago farfara. Redox Biol. 2018;18:6–15. https://doi.org/10.1016/j.redox.2018.05.015.

  27. 27.

    Zagorski JW, Turley AE, Freeborn RA, et al. Differential effects of the Nrf2 activators tBHQ and CDDO-Im on the early events of T cell activation. Biochem Pharmacol. 2018;147:67–76. https://doi.org/10.1016/j.bcp.2017.11.005.

  28. 28.

    Li S, Li J, Shen C, et al. Tert-Butylhydroquinone (tBHQ) protects hepatocytes against lipotoxicity via inducing autophagy independently of Nrf2 activation. Biochim Biophys Acta. 2014;1841(1):22–33. https://doi.org/10.1016/j.bbalip.2013.09.004.

  29. 29.

    Alexander MR, Owens GK. Epigenetic control of smooth muscle cell differentiation and phenotypic switching in vascular development and disease. Annu Rev Physiol. 2012;74:13–40. https://doi.org/10.1146/annurev-physiol-012110-142315.

  30. 30.

    Bennett MR, Sinha S, Owens GK. Vascular smooth muscle cells in atherosclerosis. Circ Res. 2016;118(4):692–702. https://doi.org/10.1161/CIRCRESAHA.115.306361.

Download references

Acknowledgements

Not applicable.

Funding

This study was supported by The Outstanding Academic Leaders Program of Shanghai Municipal Commission of Health and Family Planning (No.2017BR006), Shanghai Sailing Program Project (No.16YF1401200), and National Natural Science Foundation of China (No.81801148, No.81870911, and No.81571102).

Author information

YS contributed to the conception and design of study, collection and/or assembly of data, data analysis and interpretation, and manuscript writing. SL contributed to the database input and data interpretation, manuscript writing, and final approval of manuscript. YS contributed to the data analysis and interpretation and manuscript writing. PL contributed to the data collection, manuscript writing, and analysis. ZY and YL contributed to the animal experiments and data collection. KQ, GY, and ZF contributed to the in vitro assay data collection and analysis and histological examination. WZ contributed to the conception and design of study and revision and final approval of manuscript. WZ is the corresponding author of this article. All authors read and approved the final manuscript.

Correspondence to Wei Zhu.

Ethics declarations

Ethics approval and consent to participate

All animal procedures were carried out according to the protocol of our Institutional Animal Care and Use Committee. The experimental protocol was reviewed and approved by the Ethics Committee of the Huashan Hospital affiliated with Fudan University in Shanghai, People’s Republic of China.

Consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.

Additional information

Publisher’s Note

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Rights and permissions

Open Access This article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Keywords

  • Intracranial aneurysm
  • Nrf-2
  • Vascular smooth muscle cells phenotype
  • Oxidative stress
  • Inflammation