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A small molecule inhibitor of Nox2 and Nox4 improves contractile function after ischemia–reperfusion in the mouse heart


The NADPH oxidase enzymes Nox2 and 4, are important generators of Reactive oxygen species (ROS). These enzymes are abundantly expressed in cardiomyocytes and have been implicated in ischemia–reperfusion injury. Previous attempts with full inhibition of their activity using genetically modified animals have shown variable results, suggesting that a selective and graded inhibition could be a more relevant approach. We have, using chemical library screening, identified a new compound (GLX481304) which inhibits Nox 2 and 4 (with IC50 values of 1.25 µM) without general antioxidant effects or inhibitory effects on Nox 1. The compound inhibits ROS production in isolated mouse cardiomyocytes and improves cardiomyocyte contractility and contraction of whole retrogradely (Langendorff) perfused hearts after a global ischemia period. We conclude that a pharmacological and partial inhibition of ROS production by inhibition of Nox 2 and 4 is beneficial for recovery after ischemia reperfusion and might be a promising venue for treatment of ischemic injury to the heart.


The heart is an aerobic muscle—its contractile function is critically dependent on a continuous blood flow and an adequate supply of oxygen throughout life. These important processes are threatened in several common chronic diseases, associated with alterations in the coronary vessels, e.g., in atherosclerosis/ischemic heart disease which affects a large number of individuals and is one of the main causes of sudden death worldwide1,2. Although strong efforts are made to identify, prevent and treat contributing and confounding factors, like diabetes, hypertension and metabolic disorders, coronary atherosclerosis, conditions with cardiac ischemia/infarction and failure are still prevalent and constitute a severe burden in our society. In the acute situation, establishment of blood flow and oxygen supply to the heart is a primary goal of therapeutic interventions, but the combination of ischemia and reperfusion is a serious threat with generation of Reactive Oxygen Species (ROS) being a key pathological mechanism3,4,5,6,7. Although ROS can introduce cellular injuries, they still have beneficial effects in some organs, concentrations and time periods during an ischemia reperfusion challenge, which suggests that therapies targeting ROS should be specific, adequately dosed and introduced in a correct time period as pointed out by e.g.8.

Normal cellular processes use reactive oxygen (ROS) to maintain proper metabolism. Pathological overproduction by one or several of the specific sources of ROS is a common cause of toxic reactions and cell death. Several cellular processes can generate reactive oxygen species including the mitochondrial electron transport chain, xanthine oxidase, nitric oxide synthases, CP450, Cyclooxygenase, monoamine oxidase, NADPH oxidase family enzymes and also via succinate through reoxidation by succinate dehydrogenase (SDH) in the mitochondria9,10,11. NADPH oxidases (Nox) are a group of isoenzymes with the potential to produce large amount of ROS and may produce harmful levels of ROS when the cellular antioxidant capacity is exceeded. The Nox family enzymes are the only enzymes where production of reactive oxygen species is the primary function. To date seven members of this Nox family have been identified: Nox1, Nox2, Nox3, Nox4 Nox5, Duox1 and Doux2. Nox1, Nox2 and Nox3 have the most similarity among the isoforms, generate superoxide O2 and are activated by association with regulatory subunits12,13,14. Nox4 is widely expressed in the body and is constitutively activated and its cellular activity regulated through induced protein expression and15,16. Nox5 can be found mainly in spleen and testis and to lesser extent in other tissues of the body, e.g., tumor cells of different origin17. Hydrogen peroxide produced in excess by Nox4 contributes e.g., to glutamate mediated neurotoxicity and a number of medical conditions18,19,20,21,22. Duox 1 and 2 are regulated with Duoxa1 and 2 as well as calcium and they produce hydrogen and have originally been found in thyroid and now also in some other organs, but not in heart or brain23. Presently some of the Nox-isoforms (Nox1, Nox2 and Nox4) seem to be involved in various diseases, causative or contributing to the pathological process24,25.

In the heart, Nox2 and Nox4 are the main Nox isoforms expressed6. Nox4 has the most extensive tissue distribution and is located in endoplasmic reticulum (ER) and mitochondria and is induced by e.g., mechanical stress, hypoxia, ischemia, ER stress and mechanical stress26,27,28,29. Hypoxia inducible factor (HIF) is a main regulator at hypoxic conditions and regulates a vast number of genes and HIF is closely related to the Nox4/Nox2 activity30. The correlation of H2O2 with activation of neurofibromin 2 (NF2) and ischemia–reperfusion injury (I/R) injury indicates that this mechanism has a potential role in apoptosis of cardiomyocytes31. Although Nox activity thus seems to have an important role in the cardiac response to ischemia reperfusion challenges, the detailed function is not known. Knock down of Nox 2 using an antisense strategy attenuated hypoxia induced stress and apoptosis32. Using genetically modified animals where Nox 2 and 4 have been ablated, positive effects with reduced infarct size have been reported6, although effects were only seen in Nox 1 and 2 knockout animals in other studies33,34. The variable results from knockout animal studies suggest that full Nox inhibition might be a less successful approach and that the inhibition should be fine-tuned to have optimal effect in reducing ischemia reperfusion injury. In this study we have developed a new specific small molecule Nox2/Nox4 inhibitor (GLX481304), and show, using isolated cardiomyocytes and perfused whole hearts from mouse that the compound inhibits ROS production in the cardiac cells and improves contractility after an ischemia–reperfusion challenge.

A preliminary report of some of the results have been presented previously35.

Materials and methods

Animals and preparation

Female and male adult C57BL/6 mice were used (age 15–35 weeks, weight 20–36 g), randomly distributed into the experimental groups. Mice were maintained on a 12-h light/dark cycle and had free access to standard chow and water. Animals were euthanized with cervical dislocation according to approved procedures, the rib case opened, and a heparin/saline solution was injected in the aorta. Thereafter the heart was quickly excised, put into a beaker with cold (4 °C) Krebs–Ringer solution and transported to the experimental set-up. Cardiac perfusion was initiated within less than 7 min after euthanasia and the preparations were used for isolation of cardiomyocytes or evaluation of the contractile function in the intact heart.

Isolation of cardiomyocytes and hypoxia/reoxygenation challenge

Cardiomyocytes were isolated as described previously36. The aorta was cannulated using a Langendorff system, and the heart was perfused with 37 °C pre-warmed perfusion buffer containing 2,3-butanedione monoxime (BDM) (10 mM) for 4 min at a flow of 3 ml/min to flush blood from the vasculature and relax the muscle. Digestive enzymes were then introduced in the BDM-containing perfusion buffer with 12.5 μM Ca2+ for 10 min at 3 ml/min. The heart was removed and the atria and the right ventricle were dissected away. The left ventricle was cut in pieces with scissors and further pulled apart with forceps into small pieces. Cells were dissociated using gentle pipetting with a 5 ml plastic pipette. Digestion was stopped by adding bovine calf serum. Large tissue pieces were then filtered away with a mesh, and Ca2+ was slowly reintroduced in perfusion buffer with bovine calf serum to a final concentration of 1 mM.

The hypoxia and reoxygenation challenge of cardiomyocytes was performed at 37 °C. The freshly isolated cell suspensions were exposed to 60 min of hypoxia in glucose free, Ca2+-containing (1 mM) perfusion buffer superfused with N2/CO2 (95%/5%). The glucose free condition was introduced to make hypoxic injuries more stable and mimic ischemia in vivo37. Non-hypoxic controls were held in the same solution with glucose exposed to air for same amount of time. After the 60 min period in hypoxia or normoxia, both groups were exposed to solution equilibrated with air and held at 37 °C for another 120 min in glucose containing, Ca2+-containing (1 mM) perfusion buffer during gentle shaking every 15 min. To address the question whether the GLX481304 Nox inhibitor influenced the properties of the cardiac cells following a challenge with hypoxia-reoxygenation, cells were treated during the hypoxia reoxygenation periods as described above in the presence of 1.25 µM GLX481304 or solvent control (0.1 mM DMSO). The loading of the Reactive Oxygen Species (H2DCFDA) and Ca2+ (FLUO-4) sensors were performed immediately after the reoxygenation period and the responses recorded as described below.

Reactive oxygen species generation in stimulated cardiomyocytes

The cells were loaded for 30 min in perfusion buffer (1.0 mM Ca2+) at room temperature with the free reactive oxygen species indicator (DCF) Carboxy-H2DCFDA (5-(and-6)-carboxy-2',7'-dichlorodihydrofluorescein diacetate, 10 µM and 1% ethanol, Life Technologies, Stockholm, Sweden, cf.38). The loading was thus performed during the last 30 min of the reoxygenation period 30 min before measurements in all conditions. DCF was used since it has previously been applied extensively, including studies of cardiomyocytes39. It has some limitation due to interaction with other ROS compounds, but the sensitivity to those is much lower than for H2O240. DCF thus have limitations, as pointed out by Kalyanaraman et al.41, a way to improve the reliability in the measurements would be to include another ROS-probe e.g. the dihydroethidium (HE), but this is also associated with limitations. Dihydroethidium is fully specific for some ROS species40 but can require additional techniques (e.g. HPLC) to confirm the oxidation products41. After loading the cells were transferred to a cuvette on the stage of an inverted confocal microscope (Zeiss LSM 510 META, Carl Zeiss Microscopy GmbH, Jena, Germany) and perfused with perfusion buffer with 1 mM [Ca2+] at room temperature (22 °C). The cells were stimulated via two platinum wires in the cuvette at 0.5 Hz (0.5 ms pulse duration, supramaximal voltage using a Grass S44 stimulator and a current amplifier) and super fused with perfusion buffer (1.0 mM Ca2+). The fluorescence intensity (excitation 488, emission 522 nm) was monitored at a frame rate of ~ 0.5 Hz for ~ 10 min. The intensity changes in individual cells were evaluated. The indicator compound is converted to a fluorescent derivative by the action of free reactive oxygen species and we observed a linear increase in intensity in the cells, reflecting production of free reactive oxygen species. The slope of this increase was evaluated by linear regression as a measure of free reactive oxygen species production per unit time. To determine the amount of loaded probe in each cell, 10 µM H2O2 was added and the maximal fluorescence intensity recorded. This value was used to normalize the fluorescence increase rates. From each batch of cells (i.e. one animal) the recording procedure was performed twice in each condition (normoxia, hypoxia and hypoxia + GLX481304).

Measurement of intracellular [Ca2+] and shortening in cardiomyocytes

The cells were loaded for 30 min in perfusion buffer (1.0 mM Ca2+) at room temperature with the Ca2+ indicator FLUO-4/AM (6 µM, Life Technologies, Stockholm, Sweden), transferred to the cuvette on the confocal microscope, perfused and stimulated as described above. FLUO-4 was excited at 488 nm and the fluorescence emission recorded with a fully open pin hole using a 522 nm filter. The microscope was run in line-scan mode (frequency 25 Hz) placing the line along the long axis of the cardiomyocyte (cf. Figure 3). Approximate 30 s were recorded for each cell. The maximal fluorescence increase during stimulation (Fmax) was recorded and normalized to the relaxed value immediately before the stimulus (F0). The Fmax/ F0 ratio was considered to reflect the contraction-associated increase in intracellular [Ca2+]. The maximal extent of cell shortening during contraction was determined from the line scans and expressed in percentage of the relaxed muscle length. From each cell, 8 measurements of Fmax/F0 and 3 measurement of cell shortening were recorded and the average was taken as representative of the cell. In each experiment 11 to 21 cells were analyzed and the average was taken as representative of the experiment.

Measurement of mRNA expression with PCR

The polymerase chain reaction (PCR) was used to examine the expression of mRNA for Nox2 (forward primer CCTTTTACCTATGTGCCGGAC; reverse CATGTGATGTGTAGAGTCTTGCT) and Nox4 (forward: TGCCTGCTCATTTGGCTGT; reverse: CCGGCACATAGGTAAAAGGATG). The primers, designed for the mouse Nox forms (5–3’ direction), were obtained using the primer database Primerbank42. The products (single bands for each form) were separated on 2% agarose gels.

Measurements of contractile function of intact hearts

For in vitro measurements of cardiac contraction, a modified Langendorff setup was used43,44, with retrograde perfusion via the aorta using 37 °C Krebs–Ringer solution pre-gassed with 95%CO2/5% O2 (pH 7.4), using a peristaltic pump. The solution was recirculated, passing through filters (mesh: 5 µm after heart and 0.45 µm before the heart), with a total fluid volume of 300 ml in order to minimize the use of Nox inhibitor compound. The heart was held via the perfusion cannula in a warm chamber with humid environment. The perfusion pressure was continuously monitored and maintained at about 80 mmHg (range 80–90 mm Hg, resulting in an initial aortic/coronary flow of about 2 ml/min), by adjusting the pump speed. After the perfusion had been initiated, the left atrium was cut away and a polyethylene balloon was inserted into the left ventricle. The pressure in the ventricle was measured via the water-filled balloon connected to a pressure transducer and a data acquisition system (ADInstruments, Oxford, UK). In a preliminary series of experiments, we determined the optimal filling volume for systolic pressure. In subsequent experiments, we inflated the balloon to this volume (40 µl). All hearts were given a stabilization period of 30 min followed by an ischemia (zero perfusion) period of 30 min. During this time, perfusion was stopped and the surface of the heart was kept moist by a slow superfusion of Krebs–Ringer solution. After the ischemia period, perfusion was restarted and the cardiac function was monitored for 120 min. The hearts were paced during the experiments, except during the ischemia period, at 6 Hz (0.6 ms pulse duration, supramaximal voltage) via electrodes placed on the surface of the heart.

In initial experiments we found that a concentration of 1.25 µM of the Nox inhibitor GLX481304 could be applied without negative effects on contractile function or perfusion pressure. Higher concentrations (2.5–10 µM) resulted in a gradual decay of systolic pressure and increase of diastolic pressure. We do not know the mechanism behind these inhibitory effects at higher GLX481304 concentrations. They may relate to more extensive inhibition of Nox2 and Nox4 activity affecting cell metabolism and/or vasculature properties6,45, but we did not examine these effects further. To address the question whether the inhibitor affected the cardiac contractibility and ischemia–reperfusion responses, the hearts were thus exposed, throughout the duration of the experiment, either with Krebs–Ringer solution containing solvent (dimethyl sulfoxide, DMSO 0.1 mM) or the Nox inhibitor (1.25 µM GLX481304, dissolved in DMSO).


Krebs–Ringer solution (mM): 123 NaCl, 4.7 KCl, 1.2 MgCl2, 1.2 KH2PO4, 20 NaHCO3, 5.5 D-Glucose, 2.5 CaCl2, with pH 7.4 when oxygenated with O2/CO2 (95%/5%).

Perfusion buffer (mM): 113 NaCl, 4.7 KCl, 0.6 Na2HPO4, 1.2 MgSO4, 12 NaHCO3, 10, KHCO3, 10 Hepes, 30 Taurine, 5.5 Glucose, with pH 7.46, oxygenated with O2/CO2 (95%/5%). 2,3-Butanedione Monoxime (BDM) 10 mM was added as indicated in the text. Digestion enzymes: 0.125 mg/ml Liberase DH (Roche, Mannheim, Germany), and 0.14 mg/ml Trypsin (Gibco, Life Technologies, Stockholm, Sweden).

Identification and characterization of NOX inhibitors

GLX481304 was identified (Glucox Biotech, Stockholm, Sweden) using a high-throughput screen, selecting for inhibition of Nox4 activity utilizing a 40 000 chemically diverse library. A 348-well format assay with T-Rex-293 whole cells with inducible Nox 4 overexpression46 using Amplex Red-based assay as read-out (fluorescence) identified 728 primary hits with 50% inhibition as threshold. A counter-screen with 4 µM H2O2 and a re-test using the same assay reduced the number of hits, leaving 93 structurally diverse hits for dose–response investigation. Dose response assay selected the hits from 200 µM, 11 step threefold dilution in duplicate. This resulted in 54 hits that received an IC50 and the most potent hits around 1 µM. None of the hits demonstrated any effect of cell viability at 10 µM (Celltitre-Blue assay, resazurin, 24 h; LDH leakage assay, formazan, 3 h). GLX481304 were further characterized regarding iso-form selectivity (Nox1, Nox2 and Nox4) using whole cell assays. Nox1 in CHO cells47, Nox2 in human neutrophils48,49, Nox4 HEK 293T-Rex46 and CJ HEK 293 cells overexpressing Nox4 (purchased from Redoxis, Lund, Sweden). The latter cell type was utilized in a previous publication to determine isoform selective Nox4 activity50.

The general methods used for CJ HEK 293, HEK 293 TRex and CHO cells, were to detach the adherent cells by trypsination followed by centrifugation and washing with Hank’s balanced salt solution (HBSS) solution. Cells were then seeded in 96-well black flat-bottom plates at a density of 50,000–100,000 cells/well. All compounds were dissolved in DMSO and concentrations ranging from 0.003 to 200 μM were tested in the Nox cellular assays with a final concentration of DMSO of 1%. Cells were incubated at 37 °C with the compounds for 30 min before measurement. In the high-throughput screen HEK 293 TRex was used and tetracycline (1 mg/ml) was added 18 h before measurement to induce Nox4 expression. Production of hydrogen peroxide by Nox in intact cells was measured using Amplex red fluorescence as described47. To examine if GLX481304 inhibited Nox 1, an Amplex red based assay was used on CHO cells overexpressing Nox1 (a kind gift from Dr Vincent Jaquet, Dept. of Pathology and Immunology, Centre Médical Universitaire, Geneva, Switzerland47). The ability of GLX481304 to inhibit the iso-form Nox2 was examined using human neutrophils activated with Phorbol 12-myristate (PMA) which stimulates Nox 2 and ROS production, via a protein kinase C and nuclear factor-kappa B pathway. ROS production was determined using isoluminol, a hydrophobic luminescent compound, activated by extra cellular ROS, a reaction amplified by horseradish peroxidase7 in the assay. Luminescence after activation with 30 ng/ml PMA was detected using a Fluostar Optima microplate reader (BMG Labtech) with 1 µM Diphenyleneiodonium Chloride (DPI) as a negative control. This assay using isolated neutrophils from whole blood was performed as previously described48. To exclude any undesired redox activity GLX481304 was also tested for endogenous redox activity using 2,2-diphenyl-1-picrylhydrazyl-hydrate (DPPH, Sigma Aldrich) assay51. Solubility of the Nox inhibitors in DMSO and physiological saline (PBS) was determined using liquid chromatography and mass spectroscopy. Membrane permeability was examined using Caco-2 cell monolayers according to published protocols52. The Caco-2 cell monolayers were grown on permeable filter support and used for transport study on day 21 after seeding. Prior to the experiment a drug solution of 10 μM was prepared and warmed to 37 °C. The Caco-2 filters were washed with pre-warmed HBSS prior to the experiment, and thereafter the experiment was started by applying the donor solution on the apical side. The transport experiments were carried out at pH 6.5 in the apical chamber, reflecting the pH of the intestinal lumen, and pH 7.4 in the basolateral chamber reflecting the pH of the blood.

The experiments were performed at 37 °C and with a stirring rate of 500 rpm. The receiver compartment was sampled at 15, 30 and 60 min, and at 60 min also a final sample from the donor chamber was taken in order to calculate the mass balance of the compound. Directly after the termination of the experiment the filter inserts were washed with pre-warmed HBSS and the membrane integrity was checked. This was performed by trans-epithelial electrical resistance (TEER) measurement and by measurement of Mannitol permeability, which is a para-cellular marker used for integrity measurements.

The Caco2 study was performed by a CRO (UDOPP, BMC, and Uppsala) that have the expertise in the field of pharmacological characterization of potential pharmaceutical substances. From this study it was concluded that GLX481304 possess high membrane permeability.


All values are given as Standard Error of the Mean (SEM) with number of observations. Statistical analysis was performed using routines implemented in SigmaPlot 14 for Windows.

Ethical statement

The study is reported in accordance with ARRIVE guidelines of the European Union Council and the current laws in Sweden.

Ethics approval

All animal experiments were approved by the Regional Animal Ethical Committee (Stockholm, Sweden) and adhered to the European Community Council Directives (86/609/EEC) and approved by Stockholm’s Norra Djurförsöksetiska Nämnd.


Generation and characterization of the Nox inhibitor GLX481304

GLX481304 (Panel a, Fig. 1) was identified in a high-throughput screen using inducible overexpressed Nox4 in T-Rex-293 cells and later confirmed with another cell line (HEK 293) that constitutively overexpressed Nox4. Further examination of isoform specificity showed that GLX481304 inhibited both Nox 2 and 4 with low IC50 values, whereas it had negligible effects on Nox1 (Panel c, Fig. 1). It was also confirmed, using comparisons with a structurally closely related compound (the redox active substance GLX481369, Panel b Fig. 1) that GLX481304 did not have general antioxidant effects (Panel d, Fig. 1). We have thus shown that GLX481304 is a potent inhibitor of Nox2 and 4 without general antioxidant effects or inhibitory effects on Nox1.

Figure 1

Structure and inhibitory effects of GLX481304 Panel a and b show the chemical structure of GLX481304 and GLX481369 used as a redox control. Panel c show the IC50 values of GLX481304 for Nox 1 (open bar, in CHO cells, one technical duplicate), Nox 2 (hatched bar in human neutrophils, one technical duplicate) and Nox 4 (full bar in CJ HEK 293 cells, four measurements) isoforms. The maximal inhibition of Nox4 was 116% and the Hill coefficient 0.94. Panel d shows the antioxidant effects (Y axis shows DPPH absorbance) of the structurally related compound GLX481369 (open circles, with half maximal effect at about 2.3 µM, thin line shows fit to hyperbolic equation) and lack of effects of the GLX481304 (filled circles). The GLX481369 redox active substance was identified and disqualified as a potential Nox4 inhibitor during a SAR development to improve Nox4 inhibitors. During this development GLX481369 was later instead used as control of being a redox active substance in the selection and identification of true Nox4 inhibitors. This substance was previously also used as an internal redox control in50. Filled squares shows absorbance in DPPH without added compound and open squares the background fluorescence.

The compound GLX481304 is rapidly taken up over cell membranes in vitro and has a high protein binding ability. Cell permeability was examined using established protocols at UDOPP laboratory, (BMC Uppsala). Permeability in Caco-2 cells, using PAPP A-B assay was 7.4 ± 0.6, 10–6 cm/s. This is considered to be a high permeability. It shows no cytotoxicity in HEK 293 cells (Celltitre-Blue assay, 10 µM, 24 h and LDH Leakage assay, 10 µM, 3 h). The Cytoxity Detection Kit Plus (LDH) demonstrated 2.4% cytotoxicity during 24 h and Celltitre Blue Cell Viability assay 75% remaining viable cells for GLX481304 and 6% of the control Chloropromazine. Thus, GLX481304 demonstrated low or no cell toxicity. GLX481304 has low solubility in physiological saline (PBS, about 6 µM), but is easily dissolved in DMSO, our stock solution was 10 mM, the final concentration of DMSO in our experiments was < 0.1%.

GLX481304 inhibits generation of reactive oxygen species in isolated cardiomyocytes

We initially confirmed, using PCR (on 5 independent samples), that mRNA of both Nox 2 and Nox 4 are expressed in the mouse heart tissue, consistent with previous data26. We then explored if inhibition of Nox 2 and Nox 4 with GLX481304 affected the Reactive Oxygen Species (ROS) generation in isolated cardiomyocytes from different cell batches (i.e. animals). The cells were exposed to either normoxia (controls) or hypoxia in low glucose (mimicking ischemia) for 60 min followed by 2 h reoxygenation and exposure to glucose, and subsequently loaded with the fluorescent reactive oxygen species indicator Carboxy-H2DCFDA. A clearly increased measurable ROS production (reflecting a hypoxia/reoxygenation challenge and sufficient loading of the indicator) was observed in 3 of 6 cell batches and the effects of GLX481304 was examined in these experimental groups (including >  = 16 cells). Figure 2 shows mean values of the fluorescence increase from the indicator probe in the different conditions. Cell batches responding to the hypoxia-reoxygenation treatment with an increase in production of reactive oxygen species (hatched bar, Fig. 2), had clearly inhibited ROS production in the presence of GLX481304 (black filled bar in Fig. 2). In cells loaded with Carboxy -H2DCFDA, but not expressing high ROS, GLX481304 inhibited the ROS production slightly (grey bar, Fig. 2) compared to the non-hypoxic controls (open bar, Fig. 2). These results thus show that both Nox2 and 4 are expressed, and that inhibition of these two enzymes leads to attenuated ROS levels after a hypoxia challenge in the mouse cardiomyocytes.

Figure 2

Free Reactive Oxygen Species (ROS) production measured by rate of increase in Carboxy -H2DCFDA fluorescence in control cardiomyocytes (Ctrl, open bar, number of cells = 50) and cardiomyocytes exposed to 60 min hypoxia and 2 h reoxygenation without (Hyp. hatched bar, n = 16) and hypoxia reoxygenation in the presence of the GLX481304 (Hyp + GLX481304, filled bar, n = 23). Gray bar shows effects of GLX481304 on cell batches without hypoxia induced ROS production (n = 18). The cells were obtained from three separate batches of cell isolation, i.e. animals. Each batch was exposed to the different treatment conditions. * indicates statistical difference (P < 0.05) compared all other groups and # P < 0.05 compared to the controls. (ANOVA on log values with Holm-Sidak method for multiple comparisons).

GLX481304 improves cardiomyocyte contractility after hypoxia-reoxygenation

To address the question whether the effects of GLX481304 on reactive oxygen species production in the cardiomyocytes exposed to hypoxia-reoxygenation was accompanied by improved contractile performance we examined shortening responses and Ca2+ transients in isolated cardiomyocytes exposed to the hypoxia-reoxygenation challenge. Panel a of Fig. 3 shows an isolated control mouse cardiomyocyte with the confocal scan line used for measurements indicated. In panel b the resulting series of scan lines in a stimulated cell are shown and panel c depicts the integrated intensity changes during a series of stimulations. The hypoxia-reoxygenation challenge gave a clear reduction in cell shortening responses (Panel d). The GLX481304 Nox inhibitor significantly improved the cardiomyocyte shortening responses after the hypoxia-reoxygenation challenge. No significant change in intracellular Ca2+ levels could be seen between the groups. These data suggest that the contractile impairment after hypoxia-reoxygenation under these conditions and the beneficial effects of GLX481304 are not mediated by alterations in the Ca2+ translocation.

Figure 3

Panel a shows a confocal line scan through a control cardiomyocyte loaded with Fluo-4. Panel b shows the intensity vs time and Panel c the integrated intensity of the fluorescence signal, reflecting changes in intracellular [Ca2+]. Panel d shows shortening responses and Panel e the contraction associated increase in fluorescence of stimulated isolated cardiomyocytes exposed to normoxia (control open bar, n = 12) or hypoxia/reoxygenation without (Hyp, grey bar, n = 11–13) or with (Hyp + GLX481304, 1.25 µM, filled bar, n = 20–21). ** P < 0.01 vs both controls and Hyp + GLX481304 group (ANOVA and Holm-Sidak method).

GLX481304 improves whole heart contractility after hypoxia-reoxygenation

We evaluated the effects of the GLX481304 in the intact isolated beating heart using a Langendorff setup. Figure 4 shows an original recording of cardiac ventricular pressure (upper trace in Panel a) and perfusion pressure (lower trace in Panel a) during an in vitro ischemia–reperfusion experiment in an isolated perfused mouse heart. Immediately after mounting of the preparation the systolic (active) pressure increased and the diastolic (relaxed) pressure decreased. The values stabilized within about 15 min and initial values, prior to the ischemia (i.e. un-perfused) period, were recorded at 30 min (first arrow in Panel a of Fig. 4). When perfusion was stopped, to mimic ischemia, the active contractions ceased within a minute and after about 10 min a sustained pressure developed. When the perfusion was restarted the sustained contraction disappeared and within about 5 min, a lower diastolic pressure was established with superimposed active contractions. The diastolic and systolic pressures were recorded during two hours after the ischemia period and pressure values were determined 5 and 120 min after onset of reperfusion (second and third arrows). At the start of the experiment the perfusion pressure was adjusted to at about 90 mmHg resulting in about 2–3 ml/min perfusion. At 5 min after start of the reperfusion (2nd arrow in Panel a of Fig. 4) the perfusion pressure tended to be lower and the perfusion flow higher in the GLX481304 treated group (controls: 88.6 ± 5.1 mmHg; 2.3 ± 0.3 ml/min, n = 8; GLX481304 treated 80.9 ± 1.8 mmHg; 3.1 ± 0.24 ml/min, n = 7). The vascular resistance (calculated as pressure/flow; controls: 43.9 ± 6.6 mmHg min/ml, n = 8; GLX481304 treated 27.5 ± 2.6 mmHg min/ml, n = 7) was significantly (P < 0.05) lower in the GLX481304 group at 5 min after onset of reperfusion. At the end of the experiment, 120 min after start of reperfusion (third arrow in Panel a of Fig. 4) the perfusion pressure was slightly lower and flow slightly higher in the GLX481304 group (controls: 95.4 ± 2.7 mmHg; 1.6 ± 0.3 ml/min. n = 8; GLX481304 treated 93.6 ± 1.3 mmHg; 2.2 ± 0.3 ml/min, n = 7). The resistance values remained lower in the GLX481304 group at 120 min (controls: 78.2 ± 15.2 mmHg min/ml, n = 8; GLX481304 treated 47.8 ± 6.6 mmHg min/ml, n = 7). Although the effects of GLX481304 at 5 min after reperfusion remained to some extent for 120 min, the differences in pressure, flow and resistance were however not significant between controls and the GLX481304 this at the later time point. The results thus show that the GLX481304 treatment gave a significantly lower flow resistance with largest effects initially after the ischemia/reperfusion.

Figure 4

Effects of GLX481304 on pressure responses in Langendorff perfused mouse hearts. Panel a shows the ventricular pressure changes and panel b the perfusion pressure in the aorta of a control heart. Data were obtained at 30 min after start (arrow 1), immediately after start of reperfusion at 65 min (arrow 2) and after two hour’s reperfusion at 180 min (arrow 3). The hypoxia (non-perfused) period is 30 min (between arrows 1 and immediately before 2), followed by reperfusion. Panel b shows the diastolic pressure and panel c the developed pressure, before (arrow 1), immediately (5 min, arrow 2) and late (2 h, arrow 3) after onset of reperfusion in the non-treated control group (open bars) and in hearts receiving GLX481304 (1.25 µM, filled bars), n = 7–8. * P < 0.05 (Two Way Repeated Measures ANOVA with Holm-Sidak method for comparison).

Panel’s b and c of Fig. 4 summarizes the results from the ischemia–reperfusion experiments in the intact hearts. The diastolic pressure (Panel b) was increased after 5 min of reperfusion following the ischemia period in both the GLX481304 and the control groups. The mean values tended to be lower in the GLX481304-treated group, although no significant difference could be detected. The active developed pressure (i.e. systolic minus diastolic, Panel c) after ischemia–reperfusion was markedly decreased in the non-treated controls. In the non-treated control group the developed pressure after 5 min reperfusion was about 46% (40.1 ± 6.8 mmHg, n = 8) of the initial before the ischemia–reperfusion period. In contrast, the GLX481304-treated group was significantly (P < 0.05) less affected and the corresponding developed pressure value was about 75% (76.0 ± 12.1 mmHg, n = 8) of the initial. The developed pressure values at both 5 min and 120 min of reperfusion were significantly higher in the GLX481304 group compared to the controls. These results thus show that the presence of the GLX481304 Nox inhibitor significantly improved the contractile function and resistance to flow after an ischemia–reperfusion challenge in the isolated mouse heart.


We have identified a novel compound (GLX481304) with selective inhibitory effects on Nox 2 and 4, both expressed in mouse cardiac tissue. GLX481304, promptly reduces the free reactive oxygen species generation in cardiomyocytes and improves contractile function in cells and whole heart after a hypoxic/”ischemic “- reperfusion challenge.

Generation of Reactive Oxygen Species (ROS) via Nox enzymes is an important event in ischemia–reperfusion injury in the heart3, but the detailed pathophysiological impact of Nox activity is not fully understood, and in some aspects controversial: Significantly decreased injury following myocardial ischemia/reperfusion has been reported in Nox 1 and Nox 2 knockout mice, but not in Nox 4 deficient animals33. It has been shown34 that Nox 4 knockout decreases activation of autophagy in cardiomyocytes, an essential survival mechanism after energy stress, following glucose deprivation. Furthermore, endothelial over-expression of Nox 4 enhances endothelial vasodilation53. On the other hand6, reported that systemic knockdown of Nox 2 or systemic and cardiac knockdown of Nox 4 significantly reduced infarct size and area at risk after ischemic reperfusion challenge. Interestingly, a double knockout of Nox 2 and 4 and overexpression of a dominant negative Nox (reducing both Nox isoforms) increased the injury6. A study by54 showed that both overexpression of Nox 4 and reduced Nox activity by expression of a dominant negative forms impaired contractile function after ischemia reperfusion. Down regulation of Nox 4 using a plant derived flavonoid has also been shown to reduce chemical injury to isolated cardiomyocytes55. The available data thus suggest a complex interplay between the Nox isoforms, and that both protective and destructive processes can be initiated depending on activation state of the different enzymes, processes difficult to mimic using knockdown strategies. It thus seems logical to conclude that results from knockdown animal models of either of these enzymes are difficult to interpret and not possible to directly translate to in vivo/clinical conditions. An isoform selective and graded pharmacological inhibition of the Nox enzymes, would therefore be a more relevant approach to understand their functions and to possibly combat ischemia–reperfusion injury in heart and other tissues.

It is clearly quite a challenge to develop specific and iso-form selective NOX inhibitors. Lately four publications have been investigating the quality of several of the commonly used NOX inhibitors available today56,57,58. Several of these inhibitors investigated were found to have redox and ROS scavenging activities and/or not being iso-form selective.

Currently, few compounds selective for the different Nox isoforms are available and characterized. General inhibition can be obtained using, e.g. apocynin and diphenyleneiodonium (DPI), but these compounds are not selective for Nox and have effects on several other enzyme systems59. ML171 is presented as a NOX1 inhibitor with a 10–20 times selectivity in relation to NOX2, NOX3, NOX4, Glucose oxidase and Xanthine oxidase60,61. The mechanism of action was being questioned in one study for ML171 NOX1 inhibition62. VAS 3947 and VAS2870 have been introduced as more specific inhibitors of all Nox isoforms, but also these compounds can have off-target effects59. In spite of this imperfection VAS2870 is proposed to be a pan inhibitor63 of NOX isoforms. VAS2870 has been demonstrated to have several beneficial effects in preclinical disease models, including stroke, pulmonary hypertension, thrombosis, Alzheimer’s disease56. Compounds with isoform specificity have also been developed, e.g. the GKT136901 and GKT137831 which inhibits Nox 1 and 4. GTK137831 has been shown to rescue heart function after ischemia/reperfusion in mice64. Recently the mechanism of action regarding NOX inhibition by GKT136901 and GKT137831 have been questioned when stringent testing was performed65. GKT137831 is in spite this going through phase 2 clinical trials in diabetic nephropathy targeting NOX1/NOX4 activity. Here we show that GLX481304 in whole cell assays, expressing the NOX isoforms NOX1, NOX2 and NOX4, has a clear selectivity and GLX481304 clearly passed the test of not being redox active or ROS-scavenging.

Thus, although the detailed action of Nox inhibitors is not fully clarified, beneficial results using Nox inhibitors, e.g. DPI, Apocynin, VAS 28705,66,67 have been reported in animal models of ischemic stroke, suggesting that pharmacological inhibition of this enzyme system is a promising strategy for treating ischemic conditions in the brain. Beneficial results were also demonstrated when ML171, VAS2870 and the completely iso-form selective GLX701311450 were utilized to clarify the different roles of NOX isoforms of the pathophysiology in the retina caused by AMPA induced excitotoxicity68.

To our knowledge, studies of pharmacological Nox inhibition in ischemia/reperfusion challenge to the heart are very limited. As pointed out by Cadenas3, ROS signalling can be both protective and harmful for the heart and a carefully graded pharmacological inhibition of Nox would therefore be an attractive clinical approach to target the negative effects of ischemia/reperfusion. The specific Nox 4 inhibitor GLX7013114 has demonstrated protective effects on pancreatic islet cells and on retinal cells50,68.

The brain seems to be particularly sensitive to Nox 4 induced cytotoxicity69, but as discussed above the cardiac system might be potentially affected by both Nox 4 and 2. We therefore decided, in the present study, to target these two main Nox isoforms (2 and 4) proposed to be involved in ischemia/reperfusion injury of the heart6. Our characterization of the GLX481304 demonstrated selectivity for these two Nox isoforms and activity with IC50 values in the micromolar range.

ROS/Nox have several targets in the vascular smooth muscle and vascular endothelium53,70. However, GLX481304 clearly inhibited the up-regulated ROS in the post ischemic isolated cardiomyocytes and resulted in a significant attenuation of the ischemia induced contractile impairment, which identifies the cardiac muscle as a key target. The cardiomyocyte contraction was inhibited after the ischemia/reperfusion with lowered shortening despite normal Ca2+ transients. This implies that ROS induced inhibition in the cardiomyocytes occurs via steps down-stream of the Ca2+ increase, e.g. via effects on the cell energy metabolism, thin filament regulation or the contractile function it self. The effects of GLX481304 on ROS production in the cardiomyocytes was most pronounced after ischemia/reoxygenation whereas effects on non-upregulated ROS was lower (Fig. 2). Effects on contractility (Fig. 4) in normoxia was minimal, whereas it partially rescued cardiomyocytes and heart after hypoxia/reoxygenation (Figs. 3, 4). This suggests that the effects are mediated via effects on increased ROS production. The ROS hydrogen peroxide (H2O2) is well known as an intermediate in cellular signaling as it will bind to certain amino acids (cysteine, methionine) of proteins71. It has a long biological life span and is capable of membrane diffusion between cells72. It has been shown that reactive oxygen species reduce contractile force and reduces Ca2+ sensitivity in permeabilized pig cardiac muscle fibers, possibly by direct effects on the contractile system73. We therefore conclude that the beneficial effects of GLX481304 in the whole heart (Langendorff perfused) system are to a large extent due to direct effects on the cardiomyocytes by preventing a ROS induced modification of the contractile system.


We have shown that Nox2/Nox4 inhibition is a potentially useful pharmacological treatment of ischemia/reperfusion induced cardiac dysfunction. The inhibition of Nox2/Nox4 in the cardiac tissue using the GLX481304 is most likely only partial, a total knockout would, as previously shown in genetically modified animal, give less predictable results and possibly also reductive stress by the complete lack of Nox activity, which most likely can be as detrimental as oxidative stress. Future pharmacological treatment attempts, e.g. in myocardial ischemia/infarction, or during potential other challenges to the cardiac system including transplantation, must be performed within a therapeutic window. Our results also suggest that it is probably not necessary to have strict selectivity to one Nox isoform in the cardiac system.


  1. 1.

    Lozano, R. et al. Global and regional mortality from 235 causes of death for 20 age groups in 1990 and 2010: A systematic analysis for the Global Burden of Disease Study 2010. Lancet 380, 2095–2128. (2012).

    Article  PubMed  PubMed Central  Google Scholar 

  2. 2.

    Mehta, D., Curwin, J., Gomes, J. A. & Fuster, V. Sudden death in coronary artery disease: Acute ischemia versus myocardial substrate. Circulation 96, 3215–3223. (1997).

    CAS  Article  PubMed  Google Scholar 

  3. 3.

    Cadenas, S. ROS and redox signaling in myocardial ischemia-reperfusion injury and cardioprotection. Free Radic. Biol. Med. 117, 76–89. (2018).

    CAS  Article  PubMed  Google Scholar 

  4. 4.

    Granger, D. N. & Kvietys, P. R. Reperfusion injury and reactive oxygen species: The evolution of a concept. Redox Biol 6, 524–551. (2015).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  5. 5.

    Kleinschnitz, C. et al. Post-stroke inhibition of induced NADPH oxidase type 4 prevents oxidative stress and neurodegeneration. PLoS Biol. (2010).

    Article  PubMed  PubMed Central  Google Scholar 

  6. 6.

    Matsushima, S. et al. Broad suppression of NADPH oxidase activity exacerbates ischemia/reperfusion injury through inadvertent downregulation of hypoxia-inducible factor-1alpha and upregulation of peroxisome proliferator-activated receptor-alpha. Circ. Res. 112, 1135–1149. (2013).

    CAS  Article  PubMed  Google Scholar 

  7. 7.

    Matsushima, S., Tsutsui, H. & Sadoshima, J. Physiological and pathological functions of NADPH oxidases during myocardial ischemia-reperfusion. Trends Cardiovasc. Med. 24, 202–205. (2014).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  8. 8.

    Becker, L. B. New concepts in reactive oxygen species and cardiovascular reperfusion physiology. Cardiovasc. Res 61, 461–470. (2004).

    CAS  Article  PubMed  Google Scholar 

  9. 9.

    Chouchani, E. T. et al. Ischaemic accumulation of succinate controls reperfusion injury through mitochondrial ROS. Nature 515, 431–435. (2014).

    CAS  Article  PubMed  PubMed Central  ADS  Google Scholar 

  10. 10.

    Raedschelders, K., Ansley, D. M. & Chen, D. D. The cellular and molecular origin of reactive oxygen species generation during myocardial ischemia and reperfusion. Pharmacol. Ther. 133, 230–255. (2012).

    CAS  Article  PubMed  Google Scholar 

  11. 11.

    Sirker, A., Zhang, M. & Shah, A. M. NADPH oxidases in cardiovascular disease: Insights from in vivo models and clinical studies. Basic Res. Cardiol. 106, 735–747. (2011).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  12. 12.

    Cheng, G., Diebold, B. A., Hughes, Y. & Lambeth, J. D. Nox1-dependent reactive oxygen generation is regulated by Rac1. J. Biol. Chem. 281, 17718–17726. (2006).

    CAS  Article  PubMed  Google Scholar 

  13. 13.

    Suh, Y. A. et al. Cell transformation by the superoxide-generating oxidase Mox1. Nature 401, 79–82. (1999).

    CAS  Article  PubMed  ADS  Google Scholar 

  14. 14.

    Ueyama, T., Geiszt, M. & Leto, T. L. Involvement of Rac1 in activation of multicomponent Nox1- and Nox3-based NADPH oxidases. Mol. Cell Biol. 26, 2160–2174. (2006).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  15. 15.

    Martyn, K. D., Frederick, L. M., von Loehneysen, K., Dinauer, M. C. & Knaus, U. G. Functional analysis of Nox4 reveals unique characteristics compared to other NADPH oxidases. Cell Signal 18, 69–82. (2006).

    CAS  Article  PubMed  Google Scholar 

  16. 16.

    Nisimoto, Y., Jackson, H. M., Ogawa, H., Kawahara, T. & Lambeth, J. D. Constitutive NADPH-dependent electron transferase activity of the Nox4 dehydrogenase domain. Biochemistry 49, 2433–2442. (2010).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  17. 17.

    Antony, S. et al. Characterization of NADPH oxidase 5 expression in human tumors and tumor cell lines with a novel mouse monoclonal antibody. Free Radic. Biol. Med. 65, 497–508. (2013).

    CAS  Article  PubMed  Google Scholar 

  18. 18.

    Ha, J. S. et al. Nox4-dependent H2O2 production contributes to chronic glutamate toxicity in primary cortical neurons. Exp. Cell Res. 316, 1651–1661. (2010).

    CAS  Article  PubMed  Google Scholar 

  19. 19.

    Ha, J. S., Lim, H. M. & Park, S. S. Extracellular hydrogen peroxide contributes to oxidative glutamate toxicity. Brain Res. 1359, 291–297. (2010).

    CAS  Article  PubMed  Google Scholar 

  20. 20.

    Meldrum, B. & Garthwaite, J. Excitatory amino acid neurotoxicity and neurodegenerative disease. Trends Pharmacol. Sci. 11, 379–387. (1990).

    CAS  Article  PubMed  Google Scholar 

  21. 21.

    Meldrum, B. S. The role of glutamate in epilepsy and other CNS disorders. Neurology 44, S14-23 (1994).

    CAS  PubMed  Google Scholar 

  22. 22.

    Nishizawa, Y. Glutamate release and neuronal damage in ischemia. Life Sci. 69, 369–381. (2001).

    CAS  Article  PubMed  Google Scholar 

  23. 23.

    Ma, M. W. et al. NADPH oxidase in brain injury and neurodegenerative disorders. Mol. Neurodegen. 12, 7. (2017).

    CAS  Article  Google Scholar 

  24. 24.

    Brandes, R. P., Weissmann, N. & Schroder, K. NADPH oxidases in cardiovascular disease. Free Radic. Biol. Med. 49, 687–706. (2010).

    CAS  Article  PubMed  Google Scholar 

  25. 25.

    Cave, A. C. et al. NADPH oxidases in cardiovascular health and disease. Antioxid. Redox. Signal 8, 691–728. (2006).

    CAS  Article  PubMed  Google Scholar 

  26. 26.

    Bedard, K. & Krause, K. H. The NOX family of ROS-generating NADPH oxidases: Physiology and pathophysiology. Physiol. Rev. 87, 245–313. (2007).

    CAS  Article  PubMed  Google Scholar 

  27. 27.

    Lassegue, B., San Martin, A. & Griendling, K. K. Biochemistry, physiology, and pathophysiology of NADPH oxidases in the cardiovascular system. Circ. Res. 110, 1364–1390. (2012).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  28. 28.

    Pedruzzi, E. et al. NAD(P)H oxidase Nox-4 mediates 7-ketocholesterol-induced endoplasmic reticulum stress and apoptosis in human aortic smooth muscle cells. Mol. Cell Biol. 24, 10703–10717. (2004).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  29. 29.

    Wu, R. F., Ma, Z., Liu, Z. & Terada, L. S. Nox4-derived H2O2 mediates endoplasmic reticulum signaling through local Ras activation. Mol. Cell Biol. 30, 3553–3568. (2010).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  30. 30.

    Schodel, J. et al. High-resolution genome-wide mapping of HIF-binding sites by ChIP-seq. Blood 117, e207-217. (2011).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  31. 31.

    Matsuda, T. et al. NF2 activates hippo signaling and promotes ischemia/reperfusion injury in the heart. Circ. Res. 119, 596–606. (2016).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  32. 32.

    Yu, B., Meng, F., Yang, Y., Liu, D. & Shi, K. NOX2 antisense attenuates hypoxia-induced oxidative stress and apoptosis in cardiomyocyte. Int. J. Med. Sci. 13, 646–652. (2016).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  33. 33.

    Braunersreuther, V. et al. Role of NADPH oxidase isoforms NOX1, NOX2 and NOX4 in myocardial ischemia/reperfusion injury. J. Mol. Cell Cardiol. 64, 99–107. (2013).

    CAS  Article  PubMed  Google Scholar 

  34. 34.

    Sciarretta, S. et al. Activation of NADPH oxidase 4 in the endoplasmic reticulum promotes cardiomyocyte autophagy and survival during energy stress through the protein kinase RNA-activated-like endoplasmic reticulum kinase/eukaryotic initiation factor 2alpha/activating transcription factor 4 pathway. Circ. Res. 113, 1253–1264. (2013).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  35. 35.

    Szekeres, F., Walum, E., Wikstrom, P. & Arner, A. A small molecule inhibitor of Nox2 and Nox4 improves cardiac contractility after ischemia-reperfusion in the mouse heart. Acta Physiol. 211, 93–93 (2014).

    Google Scholar 

  36. 36.

    Dou, Y., Arlock, P. & Arner, A. Blebbistatin specifically inhibits actin-myosin interaction in mouse cardiac muscle. Am. J. Physiol. Cell Physiol. 293, C1148-1153. (2007).

    CAS  Article  PubMed  Google Scholar 

  37. 37.

    Portal, L. et al. A model of hypoxia-reoxygenation on isolated adult mouse cardiomyocytes: Characterization, comparison with ischemia-reperfusion, and application to the cardioprotective effect of regular treadmill exercise. J. Cardiovasc. Pharmacol. Ther. 18, 367–375. (2013).

    CAS  Article  PubMed  Google Scholar 

  38. 38.

    Borchi, E. et al. Role of NADPH oxidase in H9c2 cardiac muscle cells exposed to simulated ischaemia-reperfusion. J. Cell Mol. Med. 13, 2724–2735. (2009).

    Article  PubMed  Google Scholar 

  39. 39.

    Lu, S. et al. Hyperglycemia acutely increases cytosolic reactive oxygen species via O-linked GlcNAcylation and CaMKII activation in mouse ventricular myocytes. Circ. Res. 126, e80–e96. (2020).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  40. 40.

    Yang, C. et al. Analysis of hypoxia-induced metabolic reprogramming. Methods Enzymol 542, 425–455. (2014).

    CAS  Article  PubMed  Google Scholar 

  41. 41.

    Kalyanaraman, B. et al. Measuring reactive oxygen and nitrogen species with fluorescent probes: challenges and limitations. Free Radic. Biol. Med. 52, 1–6. (2012).

    CAS  Article  PubMed  Google Scholar 

  42. 42.

    Wang, X., Spandidos, A., Wang, H. & Seed, B. PrimerBank: A PCR primer database for quantitative gene expression analysis, 2012 update. Nucleic Acids Res. 40, D1144-1149. (2012).

    CAS  Article  PubMed  Google Scholar 

  43. 43.

    Balogh, J., Merisckay, M., Li, Z., Paulin, D. & Arner, A. Hearts from mice lacking desmin have a myopathy with impaired active force generation and unaltered wall compliance. Cardiovasc. Res. 53, 439–450. (2002).

    CAS  Article  PubMed  Google Scholar 

  44. 44.

    Brooks, W. W. & Apstein, C. S. Effect of treppe on isovolumic function in the isolated blood-perfused mouse heart. J. Mol. Cell Cardiol. 28, 1817–1822. (1996).

    CAS  Article  PubMed  Google Scholar 

  45. 45.

    Zhang, M., Perino, A., Ghigo, A., Hirsch, E. & Shah, A. M. NADPH oxidases in heart failure: Poachers or gamekeepers?. Antioxid Redox Signal 18, 1024–1041. (2013).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  46. 46.

    Serrander, L. et al. NOX4 activity is determined by mRNA levels and reveals a unique pattern of ROS generation. Biochem. J. 406, 105–114. (2007).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  47. 47.

    Jaquet, V. et al. NADPH oxidase (NOX) isoforms are inhibited by celastrol with a dual mode of action. Br. J. Pharmacol. 164, 507–520. (2011).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  48. 48.

    Anvari, E., Wikstrom, P., Walum, E. & Welsh, N. The novel NADPH oxidase 4 inhibitor GLX351322 counteracts glucose intolerance in high-fat diet-treated C57BL/6 mice. Free Radic. Res. 49, 1308–1318. (2015).

    CAS  Article  PubMed  Google Scholar 

  49. 49.

    Dahlgren, C. & Karlsson, A. Respiratory burst in human neutrophils. J. Immunol. Methods 232, 3–14 (1999).

    CAS  Article  Google Scholar 

  50. 50.

    Wang, X. et al. The novel NADPH oxidase 4 selective inhibitor GLX7013114 counteracts human islet cell death in vitro. PLoS ONE 13, e0204271. (2018).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  51. 51.

    Xiong, Q., Kadota, S., Tani, T. & Namba, T. Antioxidative effects of phenylethanoids from Cistanche deserticola. Biol. Pharm. Bull. 19, 1580–1585. (1996).

    CAS  Article  PubMed  Google Scholar 

  52. 52.

    Hubatsch, I., Ragnarsson, E. G. & Artursson, P. Determination of drug permeability and prediction of drug absorption in Caco-2 monolayers. Nat. Protoc. 2, 2111–2119. (2007).

    CAS  Article  PubMed  Google Scholar 

  53. 53.

    Ray, R. et al. Endothelial Nox4 NADPH oxidase enhances vasodilatation and reduces blood pressure in vivo. Arterioscler. Thromb. Vasc. Biol. 31, 1368–1376. (2011).

    CAS  Article  PubMed  Google Scholar 

  54. 54.

    Yu, Q. et al. Elimination of NADPH oxidase activity promotes reductive stress and sensitizes the heart to ischemic injury. J. Am. Heart Assoc. 3, e000555. (2014).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  55. 55.

    Wang, Y., Zhong, L., Liu, X. & Zhu, Y. Z. ZYZ-772 prevents cardiomyocyte injury by suppressing Nox4-derived ROS production and apoptosis. Molecules (2017).

    Article  PubMed  PubMed Central  Google Scholar 

  56. 56.

    Dao, V. T. et al. Isoform-selective NADPH oxidase inhibitor panel for pharmacological target validation. Free Radic. Biol. Med. 148, 60–69. (2020).

    CAS  Article  PubMed  Google Scholar 

  57. 57.

    Reis, J. et al. A closer look into NADPH oxidase inhibitors: Validation and insight into their mechanism of action. Redox. Biol. 32, 101466. (2020).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  58. 58.

    Schroder, K. NADPH oxidases: Current aspects and tools. Redox Biol. 34, 101512. (2020).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  59. 59.

    Radermacher, K. A. et al. Neuroprotection after stroke by targeting NOX4 as a source of oxidative stress. Antioxid. Redox Signal 18, 1418–1427. (2013).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  60. 60.

    Altenhofer, S., Radermacher, K. A., Kleikers, P. W., Wingler, K. & Schmidt, H. H. Evolution of NADPH oxidase inhibitors: Selectivity and mechanisms for target engagement. Antioxid. Redox. Signal 23, 406–427. (2015).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  61. 61.

    Gianni, D. et al. A novel and specific NADPH oxidase-1 (Nox1) small-molecule inhibitor blocks the formation of functional invadopodia in human colon cancer cells. ACS Chem. Biol. 5, 981–993. (2010).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  62. 62.

    Seredenina, T. et al. A subset of N-substituted phenothiazines inhibits NADPH oxidases. Free Radic. Biol. Med. 86, 239–249. (2015).

    CAS  Article  PubMed  Google Scholar 

  63. 63.

    Wingler, K. et al. VAS2870 is a pan-NADPH oxidase inhibitor. Cell. Mol. Life Sci. CMLS 69, 3159–3160. (2012).

    CAS  Article  PubMed  Google Scholar 

  64. 64.

    Yu, L. et al. Megakaryocytic leukemia 1 bridges epigenetic activation of NADPH oxidase in macrophages to cardiac ischemia-reperfusion injury. Circulation 138, 2820–2836. (2018).

    CAS  Article  PubMed  Google Scholar 

  65. 65.

    Augsburger, F. et al. Pharmacological characterization of the seven human NOX isoforms and their inhibitors. Redox Biol. 26, 101272. (2019).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  66. 66.

    Kim, J. Y., Park, J., Lee, J. E. & Yenari, M. A. NOX inhibitors—A promising avenue for ischemic stroke. Exp. Neurobiol. 26, 195–205. (2017).

    Article  PubMed  PubMed Central  Google Scholar 

  67. 67.

    Tuo, Y. H. et al. NADPH oxidase inhibitor improves outcome of mechanical reperfusion by suppressing hemorrhagic transformation. J. Neurointerv. Surg. 9, 492–498. (2017).

    Article  PubMed  Google Scholar 

  68. 68.

    Dionysopoulou, S., Wikstrom, P., Walum, E. & Thermos, K. Effect of NADPH oxidase inhibitors in an experimental retinal model of excitotoxicity. Exp. Eye Res. 200, 108232. (2020).

    CAS  Article  PubMed  Google Scholar 

  69. 69.

    Casas, A. I. et al. NOX4-dependent neuronal autotoxicity and BBB breakdown explain the superior sensitivity of the brain to ischemic damage. Proc. Natl. Acad. Sci. U.S.A. 114, 12315–12320. (2017).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  70. 70.

    Touyz, R. M. et al. Vascular smooth muscle contraction in hypertension. Cardiovasc. Res. 114, 529–539. (2018).

    CAS  Article  PubMed  PubMed Central  Google Scholar 

  71. 71.

    Holmstrom, K. M. & Finkel, T. Cellular mechanisms and physiological consequences of redox-dependent signalling. Nat. Rev. Mol. Cell Biol. 15, 411–421. (2014).

    CAS  Article  PubMed  Google Scholar 

  72. 72.

    Bienert, G. P. et al. Specific aquaporins facilitate the diffusion of hydrogen peroxide across membranes. J. Biol. Chem. 282, 1183–1192. (2007).

    CAS  Article  PubMed  Google Scholar 

  73. 73.

    Lowe, H., Baeger, I., Blasig, I. E. & Haseloff, R. F. Oxygen radicals attenuate the contractility of skinned muscle fibres from the pig myocardium. Pharmazie 49, 845–849 (1994).

    CAS  PubMed  Google Scholar 

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CJ HEK 293 cells expressing Nox4 were provided by Redoxis AB (Lund, Sweden), CHO cells expressing Nox1 from Dr Vincent Jaquet Department of Pathology and Immunology, Centre Médical Universitaire, Geneva, Switzerland.


Open access funding provided by University of Skövde. AA received support from Hans-Gabriel och Alice Trolle-Wachtmeisters Stiftelse.

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All authors contributed to the study conception and design. Material preparation, data collection and analysis were performed by F.S., A.A. and P.W. The first draft of the manuscript was written by F.S. and A.A. All authors commented on the different versions of the manuscript approved the final submitted manuscript.

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Correspondence to Ferenc L. M. Szekeres.

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PW and EW and Glucox Biotech AB have no commercial or financial interest in the Nox2/Nox4 inhibitor (GLX481304) that is used in this publication. The compound was developed by the company but is currently not patented. Both PW and EW are owner of stocks in Glucox Biotech AB. Glucox Biotech AB provided support in the form of salaries for the author PW and supplied the compound used. AA and FS have no competing interests to report.

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Szekeres, F.L.M., Walum, E., Wikström, P. et al. A small molecule inhibitor of Nox2 and Nox4 improves contractile function after ischemia–reperfusion in the mouse heart. Sci Rep 11, 11970 (2021).

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