Next Article in Journal
Modulating Nitric Oxide: Implications for Cytotoxicity and Cytoprotection
Previous Article in Journal
Ginger Polyphenols Reverse Molecular Signature of Amygdala Neuroimmune Signaling and Modulate Microbiome in Male Rats with Neuropathic Pain: Evidence for Microbiota–Gut–Brain Axis
Previous Article in Special Issue
Oxidative Stress, Antioxidants and Hypertension
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Antioxidants
Volume 13
Issue 5
10.3390/antiox13050503
antioxidants-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Article

The Vascular Function of Resistance Arteries Depends on NADPH Oxidase 4 and Is Exacerbated by Perivascular Adipose Tissue

by
Patrick Diaba-Nuhoho
†,
Jennifer Mittag
†,
Coy Brunssen
,
Henning Morawietz
* and
Heike Brendel
*
Division of Vascular Endothelium and Microcirculation, Department of Medicine III, University Hospital and Faculty of Medicine Carl Gustav Carus, TUD Dresden University of Technology, Fetscherstr. 74, 01307 Dresden, Germany
*
Authors to whom correspondence should be addressed.
†
These authors contributed equally to this study.
Antioxidants 2024, 13(5), 503; https://doi.org/10.3390/antiox13050503
Submission received: 20 March 2024 / Revised: 12 April 2024 / Accepted: 19 April 2024 / Published: 23 April 2024
(This article belongs to the Special Issue Oxidative Stress and Arterial Blood Pressure)
Browse Figures
Versions Notes

Abstract

:
The NADPH oxidase NOX4 that releases H2O2 can mediate vasoprotective mechanisms under pathophysiological conditions in conductive arteries. However, the role of NOX4 in resistance arteries and in perivascular adipose tissue is not well understood. We hypothesized that NOX4 is of functional importance in resistance arteries and perivascular adipose tissue under dyslipidemia conditions. We detected elevated NOX4 expression in murine and human vessels under dyslipidemia. Diminishing Nox4 under these conditions led to endothelial dysfunction in resistance arteries. The mesenteric arteries of Nox4−/−/Ldlr−/− mice revealed decreased eNos mRNA expression. Inhibition of eNOS in those vessels did not affect vascular function, while in Ldlr−/− mice endothelial function was significantly altered. Anticontractile properties of perivascular adipose tissue at resistance arteries were diminished in Nox4−/−/Ldlr−/− compared with Ldlr−/− mice. In addition, the presence of perivascular adipose tissue further worsened endothelial dysfunction in mesenteric arteries under dyslipidemia conditions. Perivascular adipose tissue from mesenteric arteries revealed a higher expression of markers of white adipocytes compared to markers of beige/brown adipocytes. Among those white adipocyte markers, leptin was significantly less expressed in perivascular adipose tissue from Nox4−/−/Ldlr−/− mice compared with Ldlr−/− mice. Furthermore, in human perivascular adipose tissue with a profound pattern of white adipocyte marker genes, we detected a correlation of NOX4 and LEP expression. In addition, incubating arterial vessels with leptin induced nitrite release, indicating increased eNOS activity. In humans, a higher expression of leptin in perivascular adipose tissue correlated with eNOS expression in the corresponding left internal mammary artery. In conclusion, vascular function of resistance arteries was dependent on Nox4-derived H2O2, especially under dyslipidemia conditions. Perivascular adipose tissue of the mesenteric arteries with white adipose tissue characteristics further aggravated endothelial function through reduced leptin-eNOS signaling.

1. Introduction

Dyslipidemia is one of the major risk factors for cardiovascular diseases and refers to an imbalance in serum levels of low-density lipoprotein cholesterol, high-density lipoprotein cholesterol and triglycerides, contributing to the development of atherosclerosis [1,2]. Dyslipidemia can lead to endothelial dysfunction in resistance arteries, impairing their ability to regulate blood flow and thereby contributing to hypertension and other cardiovascular complications [3]. Resistance arteries are small arteries that play a crucial role in regulating blood pressure by controlling peripheral resistance.
In the presence of dyslipidemia, the function and structure of resistance arteries can be significantly altered. The endothelium as the inner layer of a vessel wall is particularly susceptible to damage from increased levels of circulating and oxidatively modified low-density lipoproteins. This first damage, termed endothelial dysfunction, is characterized by oxidative stress and an imbalance between vasodilator and vasoconstrictor substances [4]. Consequently, endothelial dysfunction leads to increased arterial stiffness, reduced vasodilation, and impaired ability to regulate blood flow, all of which contribute to the progression of cardiovascular diseases [3]. There is evidence suggesting that the onset of endothelial dysfunction in small resistance arteries precedes the development of endothelial dysfunction in conduit arteries [5,6].
Growing evidence indicates that perivascular adipose tissue (PVAT) plays a significant role in vascular homeostasis. PVAT is a unique fat deposit surrounding many blood vessels and influences vascular function through the production and secretion of adipokines that regulate vascular tone and inflammation. Under healthy conditions, PVAT exerts anti-contractile effects that promote vasodilation [7]. PVAT might even contribute to the maintenance of endothelial function in obese patients [8]. However, in states of dyslipidemia, PVAT can become dysfunctional; its beneficial effects are diminished, and it may even contribute to the development and progression of cardiovascular diseases by secreting inflammatory cytokines and adipokines [9]. These factors promote a pro-inflammatory and pro-atherogenic environment, leading to endothelial dysfunction and vascular remodeling [10,11]. The role of the adipokine leptin in this context is not well-understood [12,13].
The NADPH oxidase (NOX) family is the predominant source of reactive oxygen species (ROS) in vessel walls. While ROS play vital roles in cellular signaling and homeostasis, excessive ROS production can lead to oxidative stress, further impairing endothelial function and promoting inflammation [14,15]. Seven NOX isoforms have been described. NOX2 generates superoxide anions and is mainly considered deleterious in the cardiovascular system. In contrast, NOX4 is the major NOX isoform in endothelial cells and mainly an enzymatic source of H2O2 instead of superoxide anions [16]. Experimental studies support the involvement of NOX4 as a secondary messenger in various biological processes including cell proliferation [17], differentiation [18], ferroptosis [19], oxygen sensing [20] and angiogenesis [21]. Additionally, NOX4 was shown to mediate vasoprotection under pathological conditions such as hypertension [22,23] and atherosclerosis [24]. Thus, NOX4 protects against the development of endothelial dysfunction and atherosclerosis in conduit arteries in LDL-receptor-deficient mice [25]. Loss of Nox4-derived H2O2 can be partially compensated for by nNOS upregulation, but severe endothelial dysfunction is not reversible. Furthermore, NOX4 mediates the protective effects of physical activity against obesity-induced vascular dysfunction. This involves NOX4-dependent exercise-induced adaptations of eNOS and Ppargc1a pathways and intracellular calcium release.
However, the role of NOX4 in small resistance arteries and in the interplay between perivascular adipose tissue and vasculature remains to be explored.

2. Materials and Methods

2.1. Mouse Models

All experiments were performed in accordance with the Guide for the Care and Use of Laboratory Animals published by the US National Institutes of Health (NIH Publication No. 85-23, revised 1996). The animal research ethics committee of the Technische Universität Dresden, Germany, and the Regional Council of Saxony (Landesdirektion Sachsen) approved the animal experiments according to institutional guidelines and German animal welfare regulations (AZ: DD24.1-5131/449/21, AZ: DD24.1-5131/449/20).
C57BL/6J/Ldlr−/− (Ldlr−/−) was obtained from The Jackson Laboratory via Charles River (Sulzfeld, Germany). C57BL/6J/Nox4−/− (Nox4−/−) mice were kindly provided by Ralf P. Brandes and Katrin Schröder (Goethe University, Frankfurt, Germany). Nox4−/−/Ldlr−/− mice were generated by crossing Nox4−/− mice with Ldlr−/− mice in-house for at least five generations and with continuous genotyping.

2.2. Human Tissue Samples

Patients were admitted to elective coronary artery bypass grafting surgery at the Heart Center Dresden, Fetscherstraße 76, 01307 Dresden, Germany. All patients received detailed verbal and written information about the study and gave written informed consent. The study was approved by the Ethics Committee of the Technische Universität Dresden (EK 307-12-2007). The investigation conforms with the principles outlined in the Declaration of Helsinki. Clinical characteristics of the patients are listed in Table 1. Dyslipidemia was defined according to the American Heart Association’s classification corresponding to the 95th percentile in an American population as total cholesterol > 5.2 mmol/L (200 mg/dL), LDL > 3.4 mmol/L (130 mg/dL), HDL < 0.9 mmol/L (35 mg/dL), or triglycerides > 1.7 mmol/L (150 mg/dL), or a combination thereof [26].
Left internal mammary artery (LIMA) and perivascular adipose tissue were dissected as described before [8]. Briefly, during coronary artery bypass graft surgery, distal remnant specimens of the left internal mammary artery were obtained from patients. The specimens were dissected approximately 30 min after sternotomy. The tissue samples were immediately stored in 25 mL TiProtec® solution (Köhler Chemie, Bensheim, Germany) at a temperature of 4 °C and transferred to the laboratory. Then the internal mammary artery was separated from perivascular tissue under a microscope and both were quickly shock frozen and stored at −80 °C for further processing.

2.3. Murine Tissue Sampling

Weight and food intake were measured before the mice were sacrificed. Animals were sacrificed by cervical dislocation; aorta, mesenteric artery, perivascular tissue from the aorta and perivascular tissue from the mesenteric artery were excised, rinsed with ice-cold PBS and snap-frozen for further analyses.

2.4. RNA Isolation and REAL-Time PCR

Tissue was lysed with RNA lysis buffer and homogenized with a Precellys homogenizer (Peqlab Biotechnologie GmbH, Erlangen, Germany). Total RNA was isolated using a peqGold Total RNA Kit (Peqlab Biotechnologie GmbH, Erlangen, Germany) and determined using a NanoDropTM 1000 Spectrophotometer (Peqlab Biotechnologie GmbH, Erlangen, Germany). Reverse transcription was performed with SuperScript II Reverse Transcriptase according to the manufacturer’s instructions (Life Technologies, Darmstadt, Germany). The mRNA expression was determined by SYBR green-based real-time PCR reactions using specific primers. Quantification was performed by real-time PCR with GoTaq qPCR Master Mix (Promega, Mannheim, Germany). Analysis of raw data was performed with 7500 Software version 2.06 (Applied Biosystems by Life Technologies, Darmstadt, Germany). Evaluation of the data was carried out using a mathematical model of relative expression ratio in real-time PCR under constant reference gene expression [27]. The primers used are listed in Table 2.

2.5. Vessel Preparation and Vascular Function Analysis

Mesenteric artery segments were isolated from the second and third branches of the mesenteric artery network, cleaned, removed and placed in Krebs-Henseleit buffer (in mM): 173.85 NaCl, 5.9 CaCl2.2H2O, 8.75 KCl, 7.4 MgSO4.7H2O, 52.5 NaHCO3, 4.1 KH2PO4 and 4.1 EDTA, with 5% CO2 in 95% O2 at 37 °C. Vascular function analysis was performed using a DMT Multi Wire Myograph System–Model 620 M (Danish Myo Technology A/S, Hinnerup, Denmark). Endothelial function was tested with acetylcholine (ACh) in rings precontracted with 1 µM phenylephrine (PE). Smooth muscle function was analyzed in precontracted rings with sodium nitroprusside (SNP). In addition, effects of ACh were tested in the presence of catalase (1500 U/mL, 30 min preincubation) or NO synthase inhibitor L-NG-Nitroarginine methyl ester (L-NAME, 300 µM, 30 min preincubation).

2.6. Griess Assay for Nitrite

Nitrite was measured using the Griess reaction. Fresh aortic vessel segments from each mouse were incubated in phenolred-free media with 10 ng/mL leptin and without. After adding 2% aminobenzenesulphoamide in 2.5% phosphoric acid, vessels were incubated for 5 min in the dark. Thereafter, 0.2% NED-reagent (N-(1-naphthyl) ethylenediamine dihydrochloride) was added and incubated and protected from light for 10 min. Absorbance at 540 nm wavelength was measured in a 96-well plate reader. With the help of a nitrite standard (0–100 µM) and linear regression, the nitrite concentration in samples was calculated. Measurements were performed in triplicate.

2.7. Serum Analysis

Serum concentrations of leptin were measured using a Mouse leptin ELISA Kit (Invitrogen, ThermoFisher Scientific, Carlsbad, CA, USA) following the manual’s instructions.

2.8. Statistical Analyses

Data are shown as mean ± standard deviation (SD). Statistical analysis was performed by a t-test or one-way ANOVA followed by the Holm–Sidak post hoc test or two-way ANOVA, respectively (GraphPad Prism 10; GraphPad Software, Inc., La Jolla, CA, USA). A value of p < 0.05 was considered statistically significant. Pearson’s correlational analysis was used and the correlation coefficient (r) was calculated.

3. Results

3.1. Increased Nox4 Expression under Dyslipidemia Conditions

In the mesenteric arteries of Ldlr−/− mice, we detected increased Nox4 mRNA expression compared with wild-type (WT) mice (Figure 1A). In human left internal mammary arteries (LIMA) from patients undergoing coronary bypass surgery, we also found evidence for higher NOX4 expression in patients with dyslipidemia (Figure 1B).

3.2. Nox4 Deletion Led to Endothelial Dysfunction in the Mesenteric Artery

To determine the impact of Nox4 in resistance vessels under dyslipidemia conditions, we analyzed the vascular function in mesenteric arteries of Ldlr−/− mice and Nox4-depleted Ldlr−/− (Nox4−/−/Ldlr−/−) mice. Endothelial dysfunction was detected in the double knockout Nox4−/−/Ldlr−/− mice (Figure 2A). Similarly, we could induce endothelial dysfunction in the mesenteric arteries of Ldlr−/− mice when incubated with H2O2 scavenger catalase, indicating the percentage of H2O2-mediated vasorelaxation in those resistance arteries (Figure 2B). We previously reported the development of endothelial dysfunction in the aorta of Nox4−/−/Ldlr−/− mice already at an age of 10 weeks. Here, we could also confirm endothelial dysfunction in the aorta of Nox4−/−/Ldlr−/− 26-week-old mice (Supplement Figure S1).
In the mesenteric artery, eNos expression was significantly decreased in Nox4−/−/Ldlr−/− mice compared with Ldlr−/− mice (Figure 2C). Consequently, incubation with nitric oxide synthase inhibitor L-NAME decreased endothelial function only in the mesenteric arteries of Ldlr−/− mice (Figure 2D), but not in the mesenteric arteries of Nox4−/−/Ldlr−/− mice. This might indicate reduced nitric oxide-mediated vasodilation in the mesenteric arteries when Nox4 is deleted (Figure 2E).

3.3. Anti-Contractile Properties of Perivascular Adipose Tissue on Mesenteric Arteries Were Absent in Nox4-Depleted Mice

In the following experiments, we analyzed the vascular function of resistance arteries with surrounding perivascular adipose tissue (PVAT). One of the key attributes of PVAT is the anti-contractile effect on the vessel. We tested that by adding potassium as well as phenylephrine to the vessel segments. Potassium-induced contraction (Figure 3A) and phenylephrine (PE)-induced contraction (Supplement Figure S2A) were significantly reduced with surrounding perivascular adipose tissue (+PVAT) in Ldlr−/− mice. In contrast, knockout of Nox4 caused increased potassium-induced contraction in mesenteric arteries with PVAT (+PVAT) (Figure 3B). The anti-contractile effect of PVAT was also absent in Nox4−/−/Ldlr−/− mice when tested with phenylephrine (Supplement Figure S2B).
Next, we analyzed endothelium-dependent vasorelaxation in the presence of PVAT. The maximal effect of acetylcholine on vasorelaxation was significantly diminished by perivascular adipose tissue (+PVAT) in Ldlr−/− mice (Figure 3C). Mesenteric arteries with perivascular adipose tissue (+PVAT) from Nox4−/−/Ldlr−/− mice showed even further decreased maximal endothelium-dependent vasorelaxation (Figure 3D).

3.4. Expression of Adipokines in Perivascular Adipose Tissue from Mesenteric Arteries of Nox4−/−/Ldlr−/− Mice and Ldlr−/− Mice and Comparison to Perivascular Adipose Tissue from Aortas

To gain a better understanding of the functional differences, we conducted comparison analysis of PVAT from mesenteric arteries of Ldlr−/− and Nox4−/−/Ldlr−/− mice. Furthermore, to evaluate the expression pattern of white and brown/beige adipocyte markers, we included PVAT from the aortas of Ldlr−/− and Nox4−/−/Ldlr−/− mice in the comparison. Expression of markers for white adipocytes significantly differed between both types of PVAT. In both mouse strains, leptin (Lep) mRNA expression was significantly higher in PVAT from mesenteric arteries compared to thoracic aorta (Figure 4A). However, PVAT from Nox4−/−/Ldlr−/− mice expressed significantly less leptin than PVAT from mesenteric arteries of Ldlr−/− mice without differences in serum leptin levels and body weight between both mouse strains (Figure 4A and Supplement Figures S3 and S4). Expression of adiponectin (Adipoq) (Figure 4B), fatty acid binding protein 4 (Fabp4) (Figure 4C) and resistin (Retn) (Figure 4D) showed a similarly higher expression in PVAT from mesenteric arteries compared with PVAT from the aorta, independent of the genotype.

3.5. Marker of Brown/Beige Adipocytes in Aortic and Mesenteric Perivascular Adipose Tissue from Nox4−/−/Ldlr−/− Mice Compared to Ldlr−/− Mice

Expression of primary indicators for brown and beige adipocytes revealed prominent expression in PVAT from the thoracic aorta and rather weak expression in PVAT from mesenteric arteries. Peroxisome proliferative-activated receptor gamma, coactivator 1 alpha (Ppargc1a) (Figure 5A) and mitochondrial brown fat uncoupling protein 1 (Ucp1) (Figure 5B) were similarly significantly elevated in murine PVAT from thoracic aortas compared with PVAT from mesenteric arteries. However, only Ucp1 was less expressed in aortic PVAT from Nox4−/−/Ldlr−/− compared with Ldlr−/− mice. In addition, brown and beige adipocyte markers bone morphogenetic protein 8b (Bmp8b) (Figure 5C), neuregulin 4 (Nrg4) (Figure 5D) and kininogen 2 (Kng2) (Figure 5E) were analyzed. We observed a similar pattern of brown/beige markers being significantly higher expressed in aortic PVAT compared with mesenteric artery PVAT. Nevertheless, we could not detect significant differences in the expression of these genes between Ldlr−/− and Nox4−/−/Ldlr−/− mice.

3.6. Adipokine Profile in Human Perivascular Adipose Tissue: Correlation of Leptin and NOX4 Expression in Human Perivascular Adipose Tissue

We were able to show severe differences in the expression of adipocyte markers with higher white adipocyte marker expression in PVAT from murine mesenteric arteries. Additionally, in those resistance arteries, we had observed that deletion of Nox4 resulted in changes in leptin expression in PVAT. To extend these findings from murine models to humans, we analyzed PVAT from human left internal mammary arteries. Here, we found a higher expression profile for white adipocyte markers including fatty acid binding protein 4 (FABP4), leptin (LEP) and adiponectin (ADIPOQ) and lower expression of brown adipocyte markers peroxisome proliferative-activated receptor gamma, coactivator 1 alpha (PPARGC1A) and uncoupling protein 1 (UCP1) (Figure 6A). Analysis of NOX4 mRNA expression and leptin (LEP) mRNA expression in human PVAT revealed a correlation, indicating a possible link between both also in humans (Figure 6B). To test the potential of leptin released by PVAT to induce eNOS activation, we exposed vessel segments to leptin in vitro and quantified nitrite concentrations in the supernatant. We detected increased nitrite concentrations as an indicator of increased nitric oxide synthase activity (Figure 6C). Finally, we were able to correlate leptin expression in the human PVAT from left internal mammary arteries with eNOS expression in the left internal arteries (Figure 6D).

4. Discussion

In the present study, we provide evidence that Nox4 is important for the maintenance of vascular function in resistance arteries under conditions of dyslipidemia. We observed increased NOX4 expression in arterial vessels from mice and humans under dyslipidemia. For human macrophages, it has already been reported that oxidized low-density lipoprotein (oxLDL) induced NOX4 expression [28]. Likewise, it has been reported that endothelial progenitor cells from hyperlipidemic patients exhibited increased NOX4 expression and activity [29]. Hypercholesterolemia is also known to induce TGF-β signaling, which in turn induces NOX4 [30,31].
On a functional level, we observed that a loss of Nox4 led to an altered endothelial function in small resistance arteries. Previously, we had reported that already in young hypercholesterolemic mice, depletion of Nox4 caused endothelial dysfunction of the aorta which further progressed after high-fat diet feeding to a higher plaque burden in the aorta [25]. Ray et al. found improved endothelium-dependent relaxation in the aorta and coronary artery of mice with endothelium-specific Nox4 overexpression [22]. It had also been shown that endothelial cells depleted of Nox4 had reduced eNos expression, Nrf-2 expression and subsequent heme oxygenase-1 expression [23]. In the mesenteric arteries of double knockout Nox4−/−/Ldlr−/− mice, we observed significantly reduced eNos expression as well. Therefore, inhibiting nitric oxide synthase in the mesenteric arteries of Nox4−/−/Ldlr−/− mice did not further impair endothelial dysfunction.
Perivascular adipose tissue (PVAT) exhibits anti-contractile properties, which we also observed in Ldlr−/− mice. However, in mice lacking Nox4, PVAT surrounding mesenteric arteries did not further decrease contractility. Additionally, PVAT on mesenteric arteries aggravated endothelial dysfunction in both Ldlr−/− and Nox4−/−/Ldlr−/− mice. Gao et al. showed that PVAT of the aorta decreased vascular contraction by releasing a factor that induced endothelium-dependent relaxation [7]. Among those factors discussed to mediate the anticontractile properties of PVAT is leptin [32]. Decreased leptin expression in perivascular adipose tissue from Nox4−/−/Ldlr−/− mice might account for the loss of anticontractile effects observed in PVAT of the mesenteric arteries in these mice. In spontaneously hypertensive rats with decreased leptin expression in their PVAT, the anticontractile effect and endothelium-dependent vasorelaxation were reduced [32]. The vasodilatory effect of leptin has also been shown in human vessels [33]. Leptin treatment of vessels from Ldlr−/− mice led to an increase in nitrite production, indicating activation of nitric oxide synthase. Leptin was reported to activate nitric oxide synthase through AKT and JAK2 [34]. However, in obesity, the mechanism might be different. Here, hyperleptinemia rather promoted eNOS uncoupling and endothelial dysfunction [35,36].
Experimental studies have shown that inhibition of NOX enzymes in adipocytes can affect leptin secretion and adipocyte differentiation [37]. Preadipocytes treated with siRNA against NOX4 exhibited fewer accumulated fat droplets. NOX4 promoted adipocyte differentiation via MAP kinase phosphatase-1 [38]. Additionally, NOX-derived reactive oxygen species have been implicated in leptin-induced effects [39,40].
In our study, comparison of the adipokine profile revealed an increased white adipocyte pattern and decreased brown/beige adipocyte marker expression in the PVAT of mesenteric arteries. In contrast, PVAT from the aorta showed increased expression of brown/beige marker genes. Mestres-Arenas et al. also observed batokines such as uncoupling protein-1 (Ucp1), peroxisome proliferator-activated receptor gamma coactivator 1-alpha (Ppargc1a), neuregulin 4 (Nrg4), kininogen-2 (Kng2) and bone morphogenetic protein-8b (Bmp8b) in murine thoracic PVAT that can even be increased by cold exposure [41].
It has been reported that leptin might stimulate β3-adrenergic receptors leading to upregulation of Ucp1 [42]. We were able to detect differences in Ucp1 expression in the more brown/beige thoracic aortic PVAT.
In human PVAT from internal mammary arteries, we observed that NOX4 expression correlated with leptin expression. Comparison of PVAT from internal mammary arteries and PVAT from coronary arteries indicated reduced leptin, IL-1β and IL-6 expression in PVAT from internal mammary arteries [43]. Thus, analyzing the effects of NOX4 in rather inflammatory PVAT might shed further light into its role in dyslipidemia, obesity, endothelial dysfunction and hypertension [14,15,44].

5. Conclusions

We provide evidence that NOX4 is essential for the vascular function of resistance arteries, particularly under dyslipidemia conditions. Deletion of Nox4 led to decreased eNOS expression and impaired nitric oxide-mediated relaxation in mesenteric arteries. We showed that PVAT under these conditions further impaired vascular function. The adipokine profile revealed decreased leptin expression and further decreased eNOS expression and activity.

6. Limitations

The focus of our investigation was the examination of resistance arteries and the perivascular adipose tissue enveloping them. Unfortunately, due to constraints in accessing human resistance arteries with perivascular adipose tissue, our analysis was restricted to internal mammary arteries with perivascular adipose tissue, thereby representing a limitation of our study. Additionally, our objectives were the investigation of Nox4-derived H2O2-mediated vasodilation and NO-mediated vasodilation specifically within resistance arteries. Nonetheless, the mechanisms underlying vasorelaxation in mesenteric arteries encompass additional factors such as prostaglandins (PGs), prostacyclin and other endothelium-derived hyperpolarizing factors (EDHFs), which, while not directly explored in this study, may differ between Ldlr−/− and Nox4−/−/Ldlr−/− mice.

Supplementary Materials

The following supporting information can be downloaded at: https://www.mdpi.com/article/10.3390/antiox13050503/s1, Supplement Figure S1: Endothelium-dependent vasorelaxation in the aorta of 26-week-old Ldlr−/− and Nox4−/−/Ldlr−/− mice; Supplement Figure S2: Phenylephrine-induced contraction in mesenteric arteries without and with perivascular adipose tissue of Ldlr−/− and Nox4−/−/Ldlr−/− mice; Supplement Figure S3: Leptin serum concentration in Ldlr−/− and Nox4−/−/Ldlr−/− mice; Supplement Figure S4: Body weight of Ldlr−/− and Nox4−/−/Ldlr−/− mice.

Author Contributions

Conceptualization, P.D.-N., C.B., H.M. and H.B.; investigation, P.D.-N., J.M. and H.B.; formal analysis, P.D.-N., J.M. and H.B.; writing—original draft preparation, P.D.-N. and H.B.; writing—review and editing, P.D.-N., J.M., C.B., H.M. and H.B.; visualization, J.M. and H.B.; supervision, H.M.; funding acquisition, P.D.-N., C.B., H.M. and H.B. All authors have read and agreed to the published version of the manuscript.

Funding

This work was supported by research grant of the German Cardiac Society (DGK) to H.B. and research grants of the Deutsche Forschungsgemeinschaft (DFG) Projektnummer 470814312 to C.B. and H.B., MO 1695/4-1 to H.M., and by the Government of Ghana and the Deutscher Akademischer Austauschdienst (91642764) to P.D.-N. We are grateful to Ralf P. Brandes and Katrin Schröder for providing us with the Nox4−/− mice.

Institutional Review Board Statement

The study was conducted in accordance with the Declaration of Helsinki. The study was approved by the Ethics Committee of the Technische Universität Dresden (EK 307-12-2007).

Informed Consent Statement

Informed consent was obtained from all patients involved in the study.

Data Availability Statement

The raw data supporting the conclusions of this article will be made available by the authors on request.

Conflicts of Interest

The authors declare no conflicts of interest.

References

  1. Berberich, A.J.; Hegele, R.A. A Modern Approach to Dyslipidemia. Endocr. Rev. 2022, 43, 611–653. [Google Scholar] [CrossRef] [PubMed]
  2. Matoba, T.; Shimokawa, H. Hydrogen peroxide is an endothelium-derived hyperpolarizing factor in animals and humans. J. Pharmacol. Sci. 2003, 92, 1–6. [Google Scholar] [CrossRef] [PubMed]
  3. Dąbrowska, E.; Narkiewicz, K. Hypertension and Dyslipidemia: The Two Partners in Endothelium-Related Crime. Curr. Atheroscler. Rep. 2023, 25, 605–612. [Google Scholar] [CrossRef]
  4. Félétou, M.; Vanhoutte, P.M. Endothelial dysfunction: A multifaceted disorder (The Wiggers Award Lecture). Am. J. Physiol. Heart. Circ. Physiol. 2006, 291, H985–H1002. [Google Scholar] [CrossRef] [PubMed]
  5. Tajima, E.; Sakuma, M.; Tokoi, S.; Matsumoto, H.; Saito, F.; Watanabe, R.; Toyoda, S.; Abe, S.; Inoue, T. The comparison of endothelial function between conduit artery and microvasculature in patients with coronary artery disease. Cardiol. J. 2020, 27, 38–46. [Google Scholar] [CrossRef] [PubMed]
  6. Berenji Ardestani, S.; Eftedal, I.; Pedersen, M.; Jeppesen, P.B.; Norregaard, R.; Matchkov, V.V. Endothelial dysfunction in small arteries and early signs of atherosclerosis in ApoE knockout rats. Sci. Rep. 2020, 10, 15296. [Google Scholar] [CrossRef]
  7. Gao, Y.-J.; Lu, C.; Su, L.-Y.; Sharma, A.M.; Lee, R.M.K.W. Modulation of vascular function by perivascular adipose tissue: The role of endothelium and hydrogen peroxide. Br. J. Pharmacol. 2007, 151, 323–331. [Google Scholar] [CrossRef]
  8. Cybularz, M.; Langbein, H.; Zatschler, B.; Brunssen, C.; Deussen, A.; Matschke, K.; Morawietz, H. Endothelial function and gene expression in perivascular adipose tissue from internal mammary arteries of obese patients with coronary artery disease. Atheroscler. Suppl. 2017, 30, 149–158. [Google Scholar] [CrossRef]
  9. Ahmed, A.; Bibi, A.; Valoti, M.; Fusi, F. Perivascular Adipose Tissue and Vascular Smooth Muscle Tone: Friends or Foes? Cells 2023, 12, 1196. [Google Scholar] [CrossRef]
  10. Stanek, A.; Brożyna-Tkaczyk, K.; Myśliński, W. The Role of Obesity-Induced Perivascular Adipose Tissue (PVAT) Dysfunction in Vascular Homeostasis. Nutrients 2021, 13, 3843. [Google Scholar] [CrossRef]
  11. Costa, R.M.; Neves, K.B.; Tostes, R.C.; Lobato, N.S. Perivascular Adipose Tissue as a Relevant Fat Depot for Cardiovascular Risk in Obesity. Front. Physiol. 2018, 9, 253. [Google Scholar] [CrossRef] [PubMed]
  12. Nosalski, R.; Guzik, T.J. Perivascular adipose tissue inflammation in vascular disease. Br. J. Pharmacol. 2017, 174, 3496–3513. [Google Scholar] [CrossRef] [PubMed]
  13. Mellott, E.; Faulkner, J.L. Mechanisms of leptin-induced endothelial dysfunction. Curr. Opin. Nephrol. Hypertens. 2023, 32, 118–123. [Google Scholar] [CrossRef] [PubMed]
  14. Amponsah-Offeh, M.; Diaba-Nuhoho, P.; Speier, S.; Morawietz, H. Oxidative Stress, Antioxidants and Hypertension. Antioxidants 2023, 12, 281. [Google Scholar] [CrossRef] [PubMed]
  15. Morawietz, H.; Brendel, H.; Diaba-Nuhoho, P.; Catar, R.; Perakakis, N.; Wolfrum, C.; Bornstein, S.R. Cross-Talk of NADPH Oxidases and Inflammation in Obesity. Antioxidants 2023, 12, 1589. [Google Scholar] [CrossRef] [PubMed]
  16. Takac, I.; Schröder, K.; Zhang, L.; Lardy, B.; Anilkumar, N.; Lambeth, J.D.; Shah, A.M.; Morel, F.; Brandes, R.P. The E-loop is involved in hydrogen peroxide formation by the NADPH oxidase Nox4. J. Biol. Chem. 2011, 286, 13304–13313. [Google Scholar] [CrossRef] [PubMed]
  17. Tang, C.-T.; Lin, X.-L.; Wu, S.; Liang, Q.; Yang, L.; Gao, Y.-J.; Ge, Z.-Z. NOX4-driven ROS formation regulates proliferation and apoptosis of gastric cancer cells through the GLI1 pathway. Cell Signal. 2018, 46, 52–63. [Google Scholar] [CrossRef] [PubMed]
  18. Hahner, F.; Moll, F.; Warwick, T.; Hebchen, D.; Buchmann, G.; Epah, J.; Abplanalp, W.; Schader, T.; Günther, S.; Gilsbach, R.; et al. Nox4 promotes endothelial differentiation through chromatin remodeling. Redox Biol. 2022, 55, 102381. [Google Scholar] [CrossRef]
  19. Park, M.W.; Cha, H.W.; Kim, J.; Kim, J.H.; Yang, H.; Yoon, S.; Boonpraman, N.; Yi, S.S.; Yoo, I.D.; Moon, J.-S. NOX4 promotes ferroptosis of astrocytes by oxidative stress-induced lipid peroxidation via the impairment of mitochondrial metabolism in Alzheimer’s diseases. Redox. Biol. 2021, 41, 101947. [Google Scholar] [CrossRef]
  20. Nisimoto, Y.; Diebold, B.A.; Constentino-Gomes, D.; Lambeth, J.D. Nox4: A hydrogen peroxide-generating oxygen sensor. Biochemistry 2014, 53, 5111–5120. [Google Scholar] [CrossRef]
  21. Craige, S.M.; Chen, K.; Pei, Y.; Li, C.; Huang, X.; Chen, C.; Shibata, R.; Sato, K.; Walsh, K.; Keaney, J.F.; et al. NADPH oxidase 4 promotes endothelial angiogenesis through endothelial nitric oxide synthase activation. Circulation 2011, 124, 731–740. [Google Scholar] [CrossRef] [PubMed]
  22. Ray, R.; Murdoch, C.E.; Wang, M.; Santos, C.X.; Zhang, M.; Alom-Ruiz, S.; Anilkumar, N.; Ouattara, A.; Cave, A.C.; Walker, S.J.; et al. Endothelial Nox4 NADPH oxidase enhances vasodilatation and reduces blood pressure in vivo. Arterioscler. Thromb. Vasc. Biol. 2011, 31, 1368–1376. [Google Scholar] [CrossRef] [PubMed]
  23. Schröder, K.; Zhang, M.; Benkhoff, S.; Mieth, A.; Pliquett, R.; Kosowski, J.; Kruse, C.; Luedike, P.; Michaelis, U.R.; Weissmann, N.; et al. Nox4 is a protective reactive oxygen species generating vascular NADPH oxidase. Circ. Res. 2012, 110, 1217–1225. [Google Scholar] [CrossRef] [PubMed]
  24. Schürmann, C.; Rezende, F.; Kruse, C.; Yasar, Y.; Löwe, O.; Fork, C.; van de Sluis, B.; Bremer, R.; Weissmann, N.; Shah, A.M.; et al. The NADPH oxidase Nox4 has anti-atherosclerotic functions. Eur. Hear. J. 2015, 36, 3447–3456. [Google Scholar] [CrossRef] [PubMed]
  25. Langbein, H.; Brunssen, C.; Hofmann, A.; Cimalla, P.; Brux, M.; Bornstein, S.R.; Deussen, A.; Koch, E.; Morawietz, H. NADPH oxidase 4 protects against development of endothelial dysfunction and atherosclerosis in LDL receptor deficient mice. Eur. Hear. J. 2016, 37, 1753–1761. [Google Scholar] [CrossRef] [PubMed]
  26. Kavey, R.E.; Daniels, S.R.; Lauer, R.M.; Atkins, D.L.; Hayman, L.L.; Taubert, K.; American Heart Association. American Heart Association guidelines for primary prevention of atherosclerotic cardiovascular disease beginning in childhood. Circulation 2003, 107, 1562–1566. [Google Scholar] [CrossRef] [PubMed]
  27. Pfaffl, M.W. A new mathematical model for relative quantification in real-time RT-PCR. Nucleic Acids Res. 2001, 29, e45. [Google Scholar] [CrossRef] [PubMed]
  28. Lee, C.F.; Qiao, M.; Schröder, K.; Zhao, Q.; Asmis, R. Nox4 is a novel inducible source of reactive oxygen species in monocytes and macrophages and mediates oxidized low density lipoprotein–induced macrophage death. Circ. Res. 2010, 106, 1489–1497. [Google Scholar] [CrossRef] [PubMed]
  29. Li, T.-B.; Zhang, Y.-Z.; Liu, W.-Q.; Zhang, J.-J.; Peng, J.; Luo, X.-J.; Ma, Q.-L. Correlation between NADPH oxidase-mediated oxidative stress and dysfunction of endothelial progenitor cell in hyperlipidemic patients. Korean J. Intern. Med. 2018, 33, 313–322. [Google Scholar] [CrossRef]
  30. Chen, P.Y.; Qin, L.; Li, G.; Wang, Z.; Dahlman, J.E.; Malagon-Lopez, J.; Gujja, S.; Cilfone, N.A.; Kauffman, K.J.; Sun, L.; et al. Endothelial TGF-beta signalling drives vascular inflammation and atherosclerosis. Nat. Metab. 2019, 1, 912–926. [Google Scholar] [CrossRef]
  31. Yan, F.; Wang, Y.; Wu, X.; Peshavariya, H.M.; Dusting, G.J.; Zhang, M.; Jiang, F. Nox4 and redox signaling mediate TGF-beta-induced endothelial cell apoptosis and phenotypic switch. Cell Death Dis. 2014, 5, e1010. [Google Scholar] [CrossRef]
  32. Gálvez-Prieto, B.; Somoza, B.; Gil-Ortega, M.; García-Prieto, C.F.; de las Heras, A.I.; González, M.C.; Arribas, S.; Aranguez, I.; Bolbrinker, J.; Kreutz, R.; et al. Anticontractile Effect of Perivascular Adipose Tissue and Leptin are Reduced in Hypertension. Front. Pharmacol. 2012, 3, 103. [Google Scholar] [CrossRef]
  33. Matsuda, K.; Teragawa, H.; Fukuda, Y.; Nakagawa, K.; Higashi, Y.; Chayama, K. Leptin causes nitric-oxide independent coronary artery vasodilation in humans. Hypertens. Res. 2003, 26, 147–152. [Google Scholar] [CrossRef]
  34. Vecchione, C.; Maffei, A.; Colella, S.; Aretini, A.; Poulet, R.; Frati, G.; Gentile, M.T.; Fratta, L.; Trimarco, V.; Trimarco, B.; et al. Leptin effect on Endothelial nitric oxide is mediated through akt–endothelial nitric oxide synthase phosphorylation pathway. Diabetes 2002, 51, 168–173. [Google Scholar] [CrossRef] [PubMed]
  35. Nakagawa, K.; Higashi, Y.; Sasaki, S.; Oshima, T.; Matsuura, H.; Chayama, K. Leptin causes vasodilation in humans. Hypertens. Res. 2002, 25, 161–165. [Google Scholar] [CrossRef]
  36. Korda, M.; Kubant, R.; Patton, S.; Malinski, T.; Tejero, J.; Shiva, S.; Gladwin, M.T.; Loria, A.S.; Spradley, F.T.; Obi, I.E.; et al. Leptin-induced endothelial dysfunction in obesity. Am. J. Physiol. Circ. Physiol. 2008, 295, H1514–H1521. [Google Scholar] [CrossRef]
  37. Castro, J.P.; Grune, T.; Speckmann, B. The two faces of reactive oxygen species (ROS) in adipocyte function and dysfunction. Biol. Chem. 2016, 397, 709–724. [Google Scholar] [CrossRef] [PubMed]
  38. Schröder, K.; Wandzioch, K.; Helmcke, I.; Brandes, R.P. Nox4 acts as a switch between differentiation and proliferation in preadipocytes. Arter. Thromb. Vasc. Biol. 2009, 29, 239–245. [Google Scholar] [CrossRef]
  39. Morawietz, H.; Bornstein, S.R. Leptin, endothelin, NADPH oxidase, and heart failure. Hypertension 2006, 47, e20, author reply e20-1. [Google Scholar] [CrossRef] [PubMed]
  40. Blanca, A.J.; Ruiz-Armenta, M.V.; Zambrano, S.; Salsoso, R.; Miguel-Carrasco, J.L.; Fortuño, A.; Revilla, E.; Mate, A.; Vázquez, C.M. Leptin Induces Oxidative Stress Through Activation of NADPH Oxidase in Renal Tubular Cells: Antioxidant Effect of L-Carnitine. J. Cell. Biochem. 2016, 117, 2281–2288. [Google Scholar] [CrossRef]
  41. Mestres-Arenas, A.; Villarroya, J.; Giralt, M.; Villarroya, F.; Peyrou, M. A Differential Pattern of Batokine Expression in Perivascular Adipose Tissue Depots From Mice. Front. Physiol. 2021, 12, 714530. [Google Scholar] [CrossRef] [PubMed]
  42. Gullicksen, P.; Flatt, W.P.; Dean, R.G.; Hartzell, D.L.; Baile, C.A. Energy metabolism and expression of uncoupling proteins 1, 2, and 3 after 21 days of recovery from intracerebroventricular mouse leptin in rats. Physiol. Behav. 2002, 75, 473–482. [Google Scholar] [CrossRef] [PubMed]
  43. Lu, D.; Wang, W.; Xia, L.; Xia, P.; Yan, Y. Gene expression profiling reveals heterogeneity of perivascular adipose tissues surrounding coronary and internal thoracic arteries. Acta Biochim. Biophys. Sin. 2017, 49, 1075–1082. [Google Scholar] [CrossRef] [PubMed]
  44. Morawietz, H. Cardiovascular protection by Nox4. Cardiovasc. Res. 2018, 114, 353–355. [Google Scholar] [CrossRef] [PubMed]
Antioxidants 13 00503 g001
Figure 1. Increased Nox4 expression under dyslipidemia conditions. (A) Relative Nox4 mRNA expression in mesenteric artery of WT compared with Ldlr−/− mice (n ≥ 7). (B) Relative NOX4 mRNA expression in left internal mammary arteries of patients without and with dyslipidemia undergoing coronary bypass surgery (n ≥ 13). Statistics: t test; * p < 0.05; ** p < 0.01.
Figure 1. Increased Nox4 expression under dyslipidemia conditions. (A) Relative Nox4 mRNA expression in mesenteric artery of WT compared with Ldlr−/− mice (n ≥ 7). (B) Relative NOX4 mRNA expression in left internal mammary arteries of patients without and with dyslipidemia undergoing coronary bypass surgery (n ≥ 13). Statistics: t test; * p < 0.05; ** p < 0.01.
Antioxidants 13 00503 g001
Antioxidants 13 00503 g002
Figure 2. Nox4 deletion led to endothelial dysfunction in mesenteric arteries of Ldlr−/− mice. (A) Concentration–response curve for acetylcholine (ACh) in mesenteric arteries of Ldlr−/− and Nox4−/−/Ldlr−/− mice (n ≥ 12). (B) Concentration–response curve for acetylcholine (ACh) in mesenteric arteries of Ldlr−/− mice with and without catalase incubation (n = 12). (C) Relative eNos mRNA expression in mesenteric arteries of Ldlr−/− and Nox4−/−/Ldlr−/− mice (n ≥ 6). (D) Concentration–response curve for acetylcholine (ACh) in mesenteric arteries of Ldlr−/− mice with and without L-NAME incubation (n ≥ 6). (E) Concentration–response curve for acetylcholine (ACh) in mesenteric arteries of Nox4−/−/Ldlr−/− mice with and without L-NAME incubation (n ≥ 10). Statistics: (A,B,D,E) sigmoidal non-linear curve fit and t test of maximal effect; (C) t test; * p < 0.05; *** p < 0.001.
Figure 2. Nox4 deletion led to endothelial dysfunction in mesenteric arteries of Ldlr−/− mice. (A) Concentration–response curve for acetylcholine (ACh) in mesenteric arteries of Ldlr−/− and Nox4−/−/Ldlr−/− mice (n ≥ 12). (B) Concentration–response curve for acetylcholine (ACh) in mesenteric arteries of Ldlr−/− mice with and without catalase incubation (n = 12). (C) Relative eNos mRNA expression in mesenteric arteries of Ldlr−/− and Nox4−/−/Ldlr−/− mice (n ≥ 6). (D) Concentration–response curve for acetylcholine (ACh) in mesenteric arteries of Ldlr−/− mice with and without L-NAME incubation (n ≥ 6). (E) Concentration–response curve for acetylcholine (ACh) in mesenteric arteries of Nox4−/−/Ldlr−/− mice with and without L-NAME incubation (n ≥ 10). Statistics: (A,B,D,E) sigmoidal non-linear curve fit and t test of maximal effect; (C) t test; * p < 0.05; *** p < 0.001.
Antioxidants 13 00503 g002
Antioxidants 13 00503 g003
Figure 3. Perivascular adipose tissue reduced contraction only in Ldlr−/− mice, but further impaired endothelium-dependent vasodilation in both Ldlr−/− and Nox4−/−/Ldlr−/− mice. (A) Potassium-induced contraction in mesenteric arteries without (-PVAT) and with perivascular adipose tissue (+PVAT) of Ldlr−/− mice (n ≥ 12). (B) Potassium-induced contraction in mesenteric arteries without (-PVAT) and with perivascular adipose tissue (+PVAT) of Nox4−/−/Ldlr−/− mice (n ≥ 9). (C) Maximal effect of concentration–response to acetylcholine (ACh) in mesenteric arteries without (-PVAT) and with perivascular adipose tissue (+PVAT) of Ldlr−/− mice (n ≥ 13). (D) Maximal effect of concentration–response to acetylcholine (ACh) in mesenteric arteries without (-PVAT) and with perivascular adipose tissue (+PVAT) of Nox4−/−/Ldlr−/− mice (n ≥ 12). Statistics: t test; * p < 0.05; ** p < 0.01.
Figure 3. Perivascular adipose tissue reduced contraction only in Ldlr−/− mice, but further impaired endothelium-dependent vasodilation in both Ldlr−/− and Nox4−/−/Ldlr−/− mice. (A) Potassium-induced contraction in mesenteric arteries without (-PVAT) and with perivascular adipose tissue (+PVAT) of Ldlr−/− mice (n ≥ 12). (B) Potassium-induced contraction in mesenteric arteries without (-PVAT) and with perivascular adipose tissue (+PVAT) of Nox4−/−/Ldlr−/− mice (n ≥ 9). (C) Maximal effect of concentration–response to acetylcholine (ACh) in mesenteric arteries without (-PVAT) and with perivascular adipose tissue (+PVAT) of Ldlr−/− mice (n ≥ 13). (D) Maximal effect of concentration–response to acetylcholine (ACh) in mesenteric arteries without (-PVAT) and with perivascular adipose tissue (+PVAT) of Nox4−/−/Ldlr−/− mice (n ≥ 12). Statistics: t test; * p < 0.05; ** p < 0.01.
Antioxidants 13 00503 g003
Antioxidants 13 00503 g004
Figure 4. Expression of adipokines in perivascular adipose tissue (PVAT) from aorta and mesenteric artery of Nox4−/−/Ldlr−/− and Ldlr−/− mice. (A) Relative leptin (Lep) mRNA expression, (B) relative adiponectin (Adipoq) mRNA expression, (C) relative fatty acid binding protein 4 (Fabp4) mRNA expression and (D) relative resistin (Retn) expression in PVAT from aorta and mesenteric artery of Ldlr−/− and Nox4−/−/Ldlr−/− mice (n ≥ 9). Statistics: two-way ANOVA; *** p < 0.001; **** p < 0.0001; ns, not significant.
Figure 4. Expression of adipokines in perivascular adipose tissue (PVAT) from aorta and mesenteric artery of Nox4−/−/Ldlr−/− and Ldlr−/− mice. (A) Relative leptin (Lep) mRNA expression, (B) relative adiponectin (Adipoq) mRNA expression, (C) relative fatty acid binding protein 4 (Fabp4) mRNA expression and (D) relative resistin (Retn) expression in PVAT from aorta and mesenteric artery of Ldlr−/− and Nox4−/−/Ldlr−/− mice (n ≥ 9). Statistics: two-way ANOVA; *** p < 0.001; **** p < 0.0001; ns, not significant.
Antioxidants 13 00503 g004
Antioxidants 13 00503 g005
Figure 5. Marker expression of brown/beige adipocytes in perivascular adipose tissue (PVAT) from aorta and mesenteric arteries of Nox4−/−/Ldlr−/− and Ldlr−/− mice. (A) Relative Pparg coactivator 1 alpha (Ppargc1a) mRNA expression, (B) relative uncoupling protein 1 (Ucp1) mRNA expression, (C) relative neuregulin 4 (Nrg4) mRNA expression, (D) relative bone morphogenetic protein 8b (Bmp8b) mRNA expression and (E) relative kininogen 2 (Kng2) mRNA expression in PVAT from aorta and mesenteric arteries of Ldlr−/− and Nox4−/−/Ldlr−/− mice (n ≥ 9). Statistics: two-way ANOVA; * p < 0.05; **** p < 0.0001; ns, not significant.
Figure 5. Marker expression of brown/beige adipocytes in perivascular adipose tissue (PVAT) from aorta and mesenteric arteries of Nox4−/−/Ldlr−/− and Ldlr−/− mice. (A) Relative Pparg coactivator 1 alpha (Ppargc1a) mRNA expression, (B) relative uncoupling protein 1 (Ucp1) mRNA expression, (C) relative neuregulin 4 (Nrg4) mRNA expression, (D) relative bone morphogenetic protein 8b (Bmp8b) mRNA expression and (E) relative kininogen 2 (Kng2) mRNA expression in PVAT from aorta and mesenteric arteries of Ldlr−/− and Nox4−/−/Ldlr−/− mice (n ≥ 9). Statistics: two-way ANOVA; * p < 0.05; **** p < 0.0001; ns, not significant.
Antioxidants 13 00503 g005
Antioxidants 13 00503 g006
Figure 6. Correlation between NOX4 and LEP mRNA expression in human perivascular adipose tissue (PVAT). (A) Relative PPARGC1A, UCP1, FABP4, LEP and ADIPOQ expression in human perivascular adipose tissue from left internal mammary arteries (LIMA). (B) Correlation of NOX4 and LEP mRNA expression in perivascular adipose tissue from left internal mammary arteries (n = 29). (C) Nitrite concentration in vessel segments from Ldlr−/− mice with and without leptin treatment (n ≥ 5). (D) Correlation of LEP mRNA expression in perivascular adipose tissue from left internal mammary arteries and eNOS expression in left internal mammary arteries (n = 30). Statistics: (C) t test; ** p < 0.01 (B,D) Pearson’s correlation coefficient (r).
Figure 6. Correlation between NOX4 and LEP mRNA expression in human perivascular adipose tissue (PVAT). (A) Relative PPARGC1A, UCP1, FABP4, LEP and ADIPOQ expression in human perivascular adipose tissue from left internal mammary arteries (LIMA). (B) Correlation of NOX4 and LEP mRNA expression in perivascular adipose tissue from left internal mammary arteries (n = 29). (C) Nitrite concentration in vessel segments from Ldlr−/− mice with and without leptin treatment (n ≥ 5). (D) Correlation of LEP mRNA expression in perivascular adipose tissue from left internal mammary arteries and eNOS expression in left internal mammary arteries (n = 30). Statistics: (C) t test; ** p < 0.01 (B,D) Pearson’s correlation coefficient (r).
Antioxidants 13 00503 g006
Table 1. Patient data: control group vs. patients with dyslipidemia. Data are shown as mean ± SD. Abbreviations: ACE, angiotensin-converting enzyme; ARB, angiotensin receptor blocker; BMI, body mass index.
Table 1. Patient data: control group vs. patients with dyslipidemia. Data are shown as mean ± SD. Abbreviations: ACE, angiotensin-converting enzyme; ARB, angiotensin receptor blocker; BMI, body mass index.
Control GroupPatients with Dyslipidemiap-Value
Number of patients1415
Dyslipidemia [yes = 1; no = 0]01
Age [years]70.07 ± 8.0271.00 ± 10.130.79
Sex [% male]100100
BMI [kg/m2]28.75 ± 3.7429.60 ± 3.280.57
Smoking [yes = 1; no = 0]0.43 ± 0.510.47 ± 0.520.84
Diabetes mellitus type 2 [yes = 1; no = 0]0.71 ± 0.470.67 ± 0.490.79
Hypertension [yes = 1; no = 0]0.93 ± 0.270.93 ± 0.260.96
Ejection fraction [%]39.67 ± 17.0839.63 ± 13.100.99
ACE inhibitor [yes = 1; no = 0]0.79 ± 0.430.60 ± 0.510.30
Beta blocker [yes = 1; no = 0]0.86 ± 0.360.93 ± 0.260.52
Statin [yes = 1; no = 0]0.86 ± 0.360.87 ± 0.350.94
Aspirin [yes = 1; no = 0]0.86 ± 0.360.87 ± 0.350.94
Diuretics [yes = 1; no = 0]0.57 ± 0.510.73 ± 0.460.38
ARB [yes = 1; no = 0]0.14 ± 0.360.20 ± 0.410.70
Table 2. Primers used for real-time PCR.
Table 2. Primers used for real-time PCR.
GenePrimersSequence, 5′-3′Accession Number
Human ADIPOQForwardTCCTCACTTCCATTCTGACTGCNM_001177800.1
ReverseGTAGAACAGCTCCCAGCAACA
Murine AdipoqForwardCAGTGGATCTGACGACACCAANM_009605.5
ReverseACGTCATCTTCGGCATGACTG
Murine Bmp8bForwardTCCGCCTATTACTGTGCTGGNM_007559.5
ReverseTAGGCACACAGCACACCTTG
Human eNOSForwardGAACCTGTGTGACCCTCACCNM_000603.5, NM_001160109.2, NM_001160110.1, NM_001160111.1
ReverseTGGCTAGCTGGTAACTGTGC
Murine eNosForwardCTCATGGGCACGGTGATGNM_008713.4
ReverseACCACATCATACTCATCCAT
Human FABP4ForwardGAAAACTGCAGCTTCCTTCTCACNM_001442.3
ReverseCTGGTGGCAAAGCCCACTC
Murine Fabp4ForwardTGGGAACCTGGAAGCTTGTCNM_001409513.1, NM_001409514.1, NM_024406.4
ReverseCTTTCCTTGTGGCAAAGCCC
Murine Kng2ForwardCGACTGCAATGCTAACGTGTNM_001102409.1, NM_001102410.1, NM_201375.2
ReverseAGGCCTCCTTCGGATAGGAAT
Human LEPForwardCAAGCTGTGCCCATCCAAAAANM_000230.2
ReverseTGAAGTCCAAACCGGTGACT
Murine LepForwardTGCTGCAGATAGCCAATGACNM_008493.3
ReverseGAGTAGAGTGAGGCTTCCAGGA
Human NOX4ForwardTAACCTCAACTGCAGCCTTATCNM_001143836.3, NM_001143837.2, NM_001291926.2, NM_001291927.1, NM_001291929.2, NM_001300995.1, NM_016931.5
ReverseCTTTTATCCAACAATCTCCTGGTTCTC
Murine Nox4ForwardTGTTGGGCCTAGGATTGTGTTNM_001285833.1, NM_001285835.1, NM_015760.5
ReverseAGGGACCTTCTGTGATCCTCG
Murine Nrg4ForwardCCTACTATCCCCAGCCCATTCTNM_032002.3, NM_001425100.1
ReverseTGCCGACAGATTACTTTCGCT
Human PPARGC1aForwardCTTTGCGCAGGTCAAACGAANM_001330753.1, NM_001330752.1, NM_013261.4, NM_001330751.1
ReverseGGTGGAAGCAGGGTCAAAGT
Murine Ppargc1aForwardAATGCAGCGGTCTTAGCACTNM_008904.2
ReverseTCTCGGTCTTAACAATGGCAGG
Human POLRIIaForwardACCTGCGGTCCACGTTGTGTNM_000937.4
ReverseCCACCATTTCCCCGGGATGCG
Murine RetnForwardTGTCCCATCGATGAAGCCATNM_001204959.1
ReverseTGGAGGAGACTGTCCAGCAA
Murine Rpl32ForwardGCGCTGCCTACGAGGTGGCTGNM_172086.2
ReverseCTGGCCCTTGAACCTTCTCCGC
Human UCP1ForwardCTAACGAAGGACCAACGGCTNM_021833.5
ReverseACGTTCCAGGATCCAAGTCG
Murine Ucp1ForwardTACCCAAGCGTACCAAGCTGNM_009463.3
ReverseACCCGAGTCGCAGAAAAGAA
Disclaimer/Publisher’s Note: The statements, opinions and data contained in all publications are solely those of the individual author(s) and contributor(s) and not of MDPI and/or the editor(s). MDPI and/or the editor(s) disclaim responsibility for any injury to people or property resulting from any ideas, methods, instructions or products referred to in the content.

Share and Cite

MDPI and ACS Style

Diaba-Nuhoho, P.; Mittag, J.; Brunssen, C.; Morawietz, H.; Brendel, H. The Vascular Function of Resistance Arteries Depends on NADPH Oxidase 4 and Is Exacerbated by Perivascular Adipose Tissue. Antioxidants 2024, 13, 503. https://doi.org/10.3390/antiox13050503

AMA Style

Diaba-Nuhoho P, Mittag J, Brunssen C, Morawietz H, Brendel H. The Vascular Function of Resistance Arteries Depends on NADPH Oxidase 4 and Is Exacerbated by Perivascular Adipose Tissue. Antioxidants. 2024; 13(5):503. https://doi.org/10.3390/antiox13050503

Chicago/Turabian Style

Diaba-Nuhoho, Patrick, Jennifer Mittag, Coy Brunssen, Henning Morawietz, and Heike Brendel. 2024. "The Vascular Function of Resistance Arteries Depends on NADPH Oxidase 4 and Is Exacerbated by Perivascular Adipose Tissue" Antioxidants 13, no. 5: 503. https://doi.org/10.3390/antiox13050503

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop