- Open Access
Apabetalone (RVX-208) reduces vascular inflammation in vitro and in CVD patients by a BET-dependent epigenetic mechanism
Clinical Epigeneticsvolume 11, Article number: 102 (2019)
Apabetalone (RVX-208) is a bromodomain and extraterminal protein inhibitor (BETi) that in phase II trials reduced the relative risk (RR) of major adverse cardiac events (MACE) in patients with cardiovascular disease (CVD) by 44% and in diabetic CVD patients by 57% on top of statins. A phase III trial, BETonMACE, is currently assessing apabetalone’s ability to reduce MACE in statin-treated post-acute coronary syndrome type 2 diabetic CVD patients with low high-density lipoprotein C. The leading cause of MACE is atherosclerosis, driven by dysfunctional lipid metabolism and chronic vascular inflammation (VI). In vitro studies have implicated the BET protein BRD4 as an epigenetic driver of inflammation and atherogenesis, suggesting that BETi may be clinically effective in combating VI. Here, we assessed apabetalone’s ability to regulate inflammation-driven gene expression and cell adhesion in vitro and investigated the mechanism by which apabetalone suppresses expression. The clinical impact of apabetalone on mediators of VI was assessed with proteomic analysis of phase II CVD patient plasma.
In vitro, apabetalone prevented inflammatory (TNFα, LPS, or IL-1β) induction of key factors that drive endothelial activation, monocyte recruitment, adhesion, and plaque destabilization. BRD4 abundance on inflammatory and adhesion gene promoters and enhancers was reduced by apabetalone. BRD2-4 degradation by MZ-1 also prevented TNFα-induced transcription of monocyte and endothelial cell adhesion molecules and inflammatory mediators, confirming BET-dependent regulation. Transcriptional regulation by apabetalone translated into a reduction in monocyte adhesion to an endothelial monolayer. In a phase II trial, apabetalone treatment reduced the abundance of multiple VI mediators in the plasma of CVD patients (SOMAscan® 1.3 k). These proteins correlate with CVD risk and include adhesion molecules, cytokines, and metalloproteinases. Ingenuity® Pathway Analysis (IPA®) predicted that apabetalone inhibits pro-atherogenic regulators and pathways and prevents disease states arising from leukocyte recruitment.
Apabetalone suppressed gene expression of VI mediators in monocytes and endothelial cells by inhibiting BET-dependent transcription induced by multiple inflammatory stimuli. In CVD patients, apabetalone treatment reduced circulating levels of VI mediators, an outcome conducive with atherosclerotic plaque stabilization and MACE reduction. Inhibition of inflammatory and adhesion molecule gene expression by apabetalone is predicted to contribute to MACE reduction in the phase III BETonMACE trial.
Vascular inflammation (VI) is a driver of atherosclerosis and is exacerbated by hypertension, hypercholesterolemia, and diabetes mellitus . Sustained high levels of circulating cytokines activate the endothelium and circulating monocytes, leading to an increase in cellular adhesion and further cytokine production. Monocytes are recruited to the activated endothelium where they adhere and transmigrate through the arterial walls (Fig. 1). Following transendothelial migration, monocytes differentiate into macrophages, taking up oxidized low-density lipoprotein (oxLDL) and forming foam cells, which leads to atherosclerotic plaque formation [2, 3]. Plaque stability itself is complex, with many contributors: infiltrating immune cells, plaque lipid and collagen content, and extracellular matrix remodeling factors . If the plaque becomes unstable and ruptures, thrombosis, stroke, or myocardial infarction (MI) can occur. One in three global deaths are estimated to be a consequence of cardiovascular disease (CVD)-related events such as these . Despite numerous pharmacological interventions, this incredible healthcare burden remains. New therapeutic strategies are needed to address the residual unmet need.
In cell nuclei, bromodomain and extraterminal (BET) proteins bind to acetylated histones and transcription factors and act as molecular scaffolds between chromatin and transcriptional machinery to regulate gene expression [6,7,8,9]. Under basal conditions, BET protein occupancy at enhancer and promoter sites on chromatin support expression of housekeeping genes important for cell maintenance and metabolism. In response to inflammatory stimuli, signaling via tumor necrosis factor receptor (TNFR), toll-like receptor (TLR), interleukin 1 receptor (IL-1R), and their respective ligands induces the translocation of the master inflammatory transcription factor nuclear factor kappa-light-chain-enhancer of activated B cells (NF-κB) from the cytoplasm to the nucleus (Fig. 2a) [10, 11]. Nuclear NF-κB binds to DNA cis-regulatory response elements at enhancers and promoters, where the NF-κB RelA/p65 subunit is acetylated . RelA acetylation recruits BRD4 from housekeeping genes to pro-inflammatory genes, forming de novo super-enhancer (SE) sites to which positive transcription elongation factor complex (P-TEFb) and chromatin remodeling factors are also recruited . Consequently, NF-κB target genes are transcribed, driving inflammation. Sustained NF-κB signaling leads to pathologies such as atherosclerosis, hypertrophy, and hypertension [13, 14].
BET inhibitors (BETi) are small molecule epigenetic modifiers with great therapeutic potential. BETi bind to the bromodomains (BD1 and BD2) of BET proteins (BRD2, BRD3, BRD4, and BRDT), preventing their interaction with acetylated lysines on histone tails and transcription factors [15,16,17]. Pan-BETi bind to BD1 and BD2 equally, while selective BETi have a greater affinity for one BD over the other. The pan-BETi JQ1 prevents inflammation-induced redistribution of BRD4 on the chromatin and suppresses tumor necrosis factor alpha (TNFα)-induced expression of inflammatory and adhesion molecules in endothelial cells [13, 14]. JQ1 also significantly reduces monocyte (THP-1 cell) adhesion to human umbilical vein endothelial cells (HUVECs) and inhibits atherogenesis in hypercholesterolemic mice . These findings highlight BETi as potential anti-inflammatory agents in atherosclerosis. Pan-BETi cannot be administered chronically due to toxic effects , and BD1-specific BETi are currently untested in humans. Therefore, it is imperative to determine whether a BD2-selective BETi maintains anti-inflammatory properties without toxicity.
Apabetalone (RVX-208) is an oral small molecule inhibitor of bromodomain and extraterminal (BET) proteins with BD2 selectivity [19, 20]. It is extremely well tolerated by patients, with safety data now exceeding 2700 patient years. The only dose-limiting toxicity observed to date is a reversible and transient elevation in alanine aminotransferases/aspartate aminotransferases in a small percentage of patients . This is managed by periodic measurement of hepatic transaminases with discontinuation of the drug if levels greater than five times the upper limit of normal are observed. This occurs in < 4% of patients in clinical trials. Further, apabetalone significantly reduced both plaque size and vulnerability (ASSURE trial) . In vitro, apabetalone has been shown to reduce pro-inflammatory gene expression in human aortic endothelial cells (HAEC) and macrophage-like U937 cells . In vivo, prophylactic and therapeutic apabetalone treatment significantly reduced aortic lesion formation and lowered levels of circulating adhesion molecules and cytokines in hyperlipidemic ApoE (−/−) mice . These findings suggest that apabetalone combats VI and has potential to reduce atherogenesis in CVD patients.
Here, we demonstrate that BET proteins are necessary for the expression of genes that drive VI and atherosclerosis. We reveal that the BD2-selective BETi, apabetalone, prevents inflammation-induced BRD4 accumulation on the enhancers and promoters of VI genes in endothelial cells. Transcription of genes involved in inflammation, endothelial dysfunction, monocyte recruitment, and plaque instability are subsequently suppressed by apabetalone treatment. This reduces the abundance of critical adhesion and monocyte recruitment proteins and functionally inhibits monocyte adhesion to inflamed endothelial cells under both static and flow conditions. We further report that apabetalone reduces the abundance of VI mediators in the plasma of CVD patients treated for 6 months (phase II trial). Our data provide a mechanism by which BD2-selective apabetalone suppresses VI through BET-dependent epigenetic transcriptional regulation. This regulation translates into a reduction in VI mediators in CVD patient plasma, which correlates with an observed reduction in plaque parameters and major adverse cardiac events (MACE).
Apabetalone inhibits BRD4 interactions with chromatin at regulatory sites in endothelial cells
The impact of apabetalone on RelA/p65 translocation and BRD4 chromatin occupancy was assessed to determine if the BD2-specific apabetalone suppresses VI transcription through the same mechanism as the pan-BETi JQ1 . In response to TNFα stimulation, phosphorylated RelA/p65 translocated from the cytoplasm to the nucleus (Fig. 3a, b) to initiate the expression of pro-inflammatory genes. Apabetalone treatment did not reduce RelA/p65 translocation (Fig. 3c); comparable levels of phospho-RelA/p65 and total RelA/p65 were measured in the nucleus of HUVECs following TNFα treatment with and without apabetalone. Further, apabetalone did not alter TNFα-induced redistribution of RelA/p65 to the enhancers and promoters of adhesion molecules or inflammatory mediators (ChIP; Fig. 3d). TNFα also increased the abundance of BRD4 bound to adhesion molecule enhancers and promoters and cytokine promoters (Fig. 3e). In contrast, apabetalone treatment suppressed the redistribution of BRD4 to these sites. Apabetalone did not alter the overall abundance of BRD4 (Additional file 1: Figure S1). These data show that the BD2-selective BETi apabetalone decreases BRD4 chromatin occupancy at regulatory sites of pro-inflammatory genes similar to the pan-BETi JQ1 . Moreover, gene transcription levels rapidly paralleled changes in BRD4 chromatin occupancy (Additional file 1: Figure S2); adhesion molecule and cytokine expression increased with TNFα treatment, and apabetalone pretreatment reduced induction to a similar extent as it reduced BRD4 chromatin occupancy.
Induction of endothelial inflammation and adhesion mediators requires BET proteins
To further demonstrate that BET proteins are necessary for VI gene expression changes, we knocked down BRD2-4 with MZ-1 in endothelial cells and assessed transcript levels after stimulus treatment (Fig. 4a). MZ-1 is a proteolysis targeting chimeric molecule (PROTAC), resulting from the fusion of the pan-BETi JQ1 and the ligand of E3 ubiquitin ligase VHL, designed to target BET proteins for ubiquitination and degradation . After confirming BRD2-4 degradation by MZ-1, we measured gene expression changes following TNFα stimulation (Fig. 4b–e). TNFα induction of endothelial adhesion molecule (Fig. 4b, c ) and cytokine (Fig. 4d, e) gene expression was largely prevented by BET protein degradation. Apabetalone pretreatment also inhibited TNFα induction of these same genes (Fig. 4b–e), albeit to a lesser extent than with MZ-1. This was expected, as non-covalent small molecule inhibitory interactions are transient in nature. These data indicate that BET proteins are required for TNFα-induced expression of key VI genes and that BD2-selective BET inhibition by apabetalone can suppress the majority of this effect.
Apabetalone represses cytokine and endotoxin induction of multiple VI mediator transcripts in endothelial cells
Widespread inflammatory responses that converge on NF-κB signaling (Fig. 2a) are key drivers of VI. To examine if apabetalone can disrupt these responses, we treated endothelial cells with TNFα, interleukin 1 beta (IL-1β), or lipopolysaccharide (LPS) and assessed gene expression (Table 1). The stimulants differentially induced HUVEC transcription of multiple cytokines, chemokines, TLR signaling molecules, and adhesion molecules. For instance, TNFα robustly induced E-selectin (SELE) over 1000 fold, while IL-1β increased expression ~ 370 fold and LPS 11 fold. Regardless of the extent of induction, however, apabetalone treatment suppressed the effects of each stimulant tested (Table 1), highlighting the central role BET proteins play in endothelial cell responses to inflammatory stimuli that activate NF-κB signaling.
To obtain a broader endothelial gene expression data set for bioinformatic analysis, we used the NanoString nCounter® Inflammation V2 gene expression panel (NanoString Technologies) to simultaneously assay expression of 255 genes. TNFα induced 109 genes by more than 1.3 fold (data not shown). Apabetalone suppressed the induction of 79 of those 109 transcripts, including chemokines, cytokines, transcription factors, receptors, and enzymes. Differences in absolute induction and reduction between data sets were the result of differences in assay sensitivities (Tables 1 and 2). The overlap in regulated genes, however, was extensive. Ingenuity® Pathway Analysis (IPA®) was used to predict endothelial upstream regulators, canonical pathways, and diseases and biological functions increased by TNFα (positive activation z-score> ~ 2) and inhibited by apabetalone treatment (negative activation z-score < ~ − 2). Predicted upstream regulators included the endotoxin LPS, cytokines, and TLR signaling molecules (Table 3). IPA® also predicted inhibition of multiple pro-inflammatory canonical pathways, including interleukin 6 (IL-6), NF-κB, and high mobility group box 1 (HMGB1) signaling, by apabetalone (Table 4). IPA® diseases and biological functions analysis highlighted processes involved in immune cell activation, movement, and recruitment as potentially counteracted by apabetalone (Table 5). Many of the endothelial genes repressed by apabetalone are associated with atherogenesis [25, 26]; their suppression is predicted to suppress atherosclerotic progression.
BET proteins are necessary for induction of inflammation and adhesion mediator transcripts in monocytes
Confirmation of the central role of BET proteins in the expression of key inflammatory and adhesion molecules in monocytes was completed by treating THP-1 cells with MZ-1 and apabetalone and assessing subsequent gene expression changes. TNFα induction of monocyte genes is subtle compared to the response of endothelial cells. However, TNFα did upregulate THP-1 expression of several key VI mediators (Fig. 5; Table 6). This response is BET protein dependent; BET protein degradation (Fig. 5a) abolished the induction of IL-1β (Fig. 5b), monocyte chemoattractant protein (MCP-1) (Fig. 5c), and innate immune signal transduction adaptor (MYD88) (Fig. 5d). Apabetalone also suppressed the expression of these same monocyte genes (Fig. 5b–d) and the transcription of several other cytokine, chemokine, TLR signaling, and adhesion molecules (Table 6). Thus, BET proteins are required for the induction of pro-atherogenic and VI-related gene expression in both monocytes and endothelial cells, and targeted inhibition by apabetalone suppresses transcription in each cell type.
Repression of transcription by apabetalone decreases the abundance of endothelial VI proteins
To determine if apabetalone’s transcriptional repression of VI mediators translated into a reduction in VI protein abundance, we quantified adhesion molecules on the surface of endothelial cells and chemokine release in response to treatment by flow cytometry. TNFα stimulation significantly increased the abundance of surface adhesion molecules (Fig. 6a, b, c) and evoked endothelial chemokine release (Fig. 6d). Apabetalone significantly reduced the percentage of HUVEC cells expressing vascular cell adhesion molecule 1 (VCAM-1) (Fig. 6a, b) and suppressed its surface abundance for more than 5 fold (Fig. 6c). SELE, an early adhesion marker for leukocyte recruitment, was also inhibited by apabetalone but to less extent than VCAM-1. Apabetalone resulted in a small but significant decrease of HUVEC expressing SELE proportional to the induced condition (Fig. 6b). The subtle change leads to a trending drop in SELE surface levels (Fig. 6c, p = 0.1). Endothelial secretion of MCP-1 was suppressed by apabetalone treatment (Fig. 6d). Overall, observations made at the gene transcript level largely translated into changes in protein expression.
Monocyte adhesion to endothelial cells is suppressed by apabetalone
Monocyte adhesion to stimulated endothelial cells was quantified to investigate if apabetalone functionally alters adhesion under static or flow conditions. In both experiments, an endothelial monolayer was pretreated with BETi for 1 h before being additionally stimulated with TNFα for 4 h. In the static experiment, monocytes were allowed to sediment onto the endothelial monolayer for 1 h before non-adherent cells were removed and adhesion was quantified (Fig. 7a). BETi pretreatment of HUVECs resulted in the adherence of fewer monocytes (Fig. 7b). To increase the clinical relevance of the experiment, monocytes were perfused over a HAEC monolayer and adhesion was quantified (Fig. 7c). BETi pretreatment of HAECs also suppressed monocyte adhesion under flow (Fig. 7d). Remarkably, 0.2 μM JQ1 and 5 μM apabetalone, BETi with distinct chemical scaffolds and pan vs BD2 selectivity, had comparable effects, reducing adhesion by 35% (Fig. 7d). These data demonstrate that the BD2-selective BETi apabetalone does inhibit monocyte adhesion to endothelial cells, an early step in the atherogenic process.
Apabetalone lowers the abundance of pro-atherogenic proteins in ASSURE CVD patient plasma
To determine the clinical effect of apabetalone on circulating protein abundance, SOMAscan™ 1.3K quantified the relative amount of ~ 1300 proteins in the plasma of ASSURE CVD patients treated with placebo (n = 47) or apabetalone (n = 47) for 26 weeks . IPA® was used to predict upstream regulators, canonical pathways, and diseases and biological functions altered by apabetalone. Only proteins whose abundance changed by more than 10% with a p value less than 0.05 in apabetalone vs placebo-treated patients were included in this analysis. IPA® predicted inhibition of multiple pro-inflammatory upstream regulators by apabetalone treatment (Table 7, z-score <− 2), including macrophage migration inhibitory factor (MIF), TNFα, CD40 ligand (CD40LG), IFNγ, IL-6, granulocyte-macrophage colony stimulating factor (CSF-2/GM-CSF), and IL-1β. Interestingly, TNFα, IL-1β, IFNγ and IL-6 were also identified as upstream regulators in the endothelial gene expression data set analysis (Table 3). In plasma, apabetalone suppressed the abundance of many TNFα, IL-6, and IL-1β target proteins that correlate with CVD risk (Table 8). These include pro-inflammatory mediators and adhesion proteins that contribute to atherogenesis, and matrix metalloproteinases implicated in plaque instability. IPA® also predicted inhibition of the canonical “HMGB1 signaling” pathway by apabetalone in the analysis of both the patient plasma (Table 7) and endothelial cell data sets (Table 4). IPA® of the CVD patient plasma proteome further highlighted diseases and biological functions predicted to be inhibited by apabetalone (Table 9). The majority have strong immune cell activation, interaction, and recruitment components that are directly associated with VI and atherogenesis (Table 9). This data indicates that the BD2-selective BETi apabetalone lowers the abundance of VI mediators that play important roles in inflammation, vascular adhesion, and plaque stability in CVD patients.
In CVD and T2DM, elevated circulating cytokines potentiate VI through recruitment of leukocytes to the vascular endothelium. BET proteins are essential VI transcriptional regulators. Recent reports have demonstrated that pan-BETi and BRD2-4 siRNA prevent an increase in endothelial VI gene expression in response to inflammation [13, 28]. Here, we extend those findings, showing that MZ-1 degradation of BRD2-4 in both monocytes and endothelial cells suppresses TNFα induction of VI gene transcription.
Moreover, the BD2-selective BETi apabetalone has a similar impact on VI transcription as a pan-BETi: apabetalone treatment inhibits transcription by preventing BRD4 accumulation on VI gene enhancers and promoters. Transcriptional regulation by apabetalone critically reduces the abundance of surface adhesion molecules, impairing monocyte adhesion to stimulated endothelial cells. We also present clinical evidence that a BD2-selective BETi regulates circulating VI proteins. Analysis of the CVD patient plasma from the ASSURE phase II trial reveals that apabetalone treatment for 26 weeks reduces the abundance of multiple VI mediators. These mediators are involved in monocyte recruitment, adhesion, macrophage differentiation, and plaque stability, highlighting the clinical impact apabetalone has on VI.
Atherosclerosis contributes significantly to coronary artery disease, the leading cause of death in the developed world . It is the combined consequence of chronic VI and lipid metabolism dysfunction, characterized by abnormally elevated levels of low-density lipoprotein (LDL) in the blood. Sub-endothelial retention of LDL, particularly oxLDL, is an initiating event in atherogenesis  and a contributing factor in plaque development . However, combating rising LDL levels alone with HMG-CoA reductase inhibitors (statins) has failed to completely eliminate MACE events due to atherosclerosis . Despite LDL management, approximately 1/3 of all CVD patients on statins still experience cardiovascular events due to residual inflammation . Compounds that inhibit hyper-inflammatory signaling or block leukocyte-endothelial interactions are now being developed to combat residual inflammatory risk in atherosclerosis. For instance, direct suppression of inflammation with an interleukin IL-1β monoclonal antibody (canakinumab) reduced the relative risk of MACE by 15% in CVD patients over 3.7 years . The Canakinumab Anti-Inflammatory Thrombosis Outcomes Study (CANTOS) has demonstrated that inflammation is another viable therapeutic target for the prevention of CVD-related events. The BD2-selective BETi apabetalone has also been shown to significantly reduce the relative risk of MACE. This may be attributed to its suppression of inflammatory gene expression and transcription of genes key to atherogenesis. These genes contribute to monocyte activation and recruitment, leukocyte capture, rolling, adhesion, firm adhesion, macrophage differentiation, plaque development, and stability (Fig. 1).
Inflammation and monocyte recruitment
Apabetalone’s impact on inflammation is extensive, inhibiting the transcription of multiple chemokines/cytokines, cognate receptors, and components upstream of NF-κB activation (Fig. 2b). MCP-1, a chemokine secreted by both endothelial cells  and monocytes , is a key attractant in monocyte recruitment (Fig. 1). Previous studies have demonstrated that MCP-1 deficiency reduces atherosclerosis in ApoE (−/−) or LDLr (−/−) murine models  and that apabetalone inhibits TNFα-induced MCP-1 gene expression in HAEC endothelial cells . Here, we demonstrate that BET proteins are required for the induction of MCP-1 transcription in endothelial cells and monocytes and that a BD2-specific BETi regulates MCP-1 expression by displacing BRD4 from its promoter. Consequently, endothelial cells secrete less MCP-1. Apabetalone also reduces monocyte C-C motif chemokine receptor 2 (CCR2) expression, the cognate receptor of MCP-1. Through its reduction of both MCP-1 and CCR2, apabetalone treatment can be expected to reduce monocyte recruitment. Apabetalone also inhibits the transcription of major pro-inflammatory mediators that converge on NF-κB signaling through the TNFR, TLR, and IL-1R signaling pathways (Fig. 2). IPA® predicted that each of these pathways was regulated in apabetalone treated endothelial cells (NanoString) (Table 3). Functionally, apabetalone’s inhibition of these mediators is predicted by IPA® to inhibit immune cell activation, migration, and chemotaxis induced by TNFα stimulation (Table 5).
Leukocyte capture, the next step in atherogenesis, relies on endothelial cell surface expression of selectins (P-selectin and SELE) (Fig. 1) . These adhesion molecules bind to leukocyte surface glycosylated ligands with high affinity in the presence of flow (shear stress) due to the “catch-bond” phenomenon [25, 37, 38]. Induction of SELE transcription not only requires BET proteins (Fig. 4c), it is the consequence of increased BRD4 occupancy on the SELE enhancer and promoter (Fig. 3e). Apabetalone inhibits SELE expression whether it is induced by TNFα, IL-1β, or LPS (Table 1). At the protein level, TNFα induction of SELE was variable, with apabetalone treatment resulting in a trending decrease in abundance (p = 0.1; Fig. 6b). These data indicate that apabetalone may impede early capture of monocytes by downregulating SELE expression.
Slow leukocyte rolling and firm adhesion
Slow leukocyte rolling and firm adhesion follow initial capture and depend on leukocyte integrin (β2-integrin, Very Late Antigen-4 (VLA-4)) interactions with endothelial adhesion molecules (e.g., VCAM-1) (Fig. 1). VCAM-1 is only expressed in activated or dysfunctional endothelial cells in pro-atherogenic regions and areas in vessels where lesions are already established [39,40,41]. VCAM-1 interactions with monocyte VLA-4 are potentiated by “inside-out” and “outside-in” signaling, establishing firm adhesion and initiating the formation of docking structures [39, 42,43,44]. VCAM-1/VLA-4 binding also triggers the junction opening process, a requirement for trans-endothelial migration [25, 43, 45]. Previous studies have shown that treatment with anti-VCAM-1 antibody inhibits leukocyte adhesion, attenuates atherosclerosis, decreases plaque inflammation, and improves plaque stability in ApoE (−/−) mice . In CVD patients, circulating levels of soluble VCAM-1 correlate positively with measures of carotid intima-media thickness and plaque destabilization [47, 48]. VCAM-1 gene expression was inhibited by apabetalone treatment of endothelial cells in vitro and in ApoE (−/−) mice carotid arteries . Here, we show that apabetalone regulates VCAM-1 transcription through a BET-dependent mechanism in endothelial cells, and VCAM-1 surface abundance is substantially reduced as an outcome (Fig. 6a). In ASSURE CVD patient plasma, VCAM-1 protein abundance was also reduced by apabetalone treatment (12.2%, p = 0.005, vs placebo; Table 8). Firm adhesion is further compromised by apabetalone’s reduction of monocyte VLA-4 transcripts that encode VCAM-1’s cognate receptor (Table 6). Thus, apabetalone is predicted to alter slow leukocyte rolling and firm adhesion by downregulating VCAM-1 and VLA-4 expression. Furthermore, here we show that in vitro, apabetalone does suppress monocyte adhesion to a TNFα stimulated endothelial monolayer under both static and flow conditions (Fig. 7), underscoring the functional consequence of BET-dependent inhibition on firm adhesion.
Firm adhesion also relies on interleukin 8 (IL-8) signaling . IL-8 release from endothelial cells attracts leukocytes and neutrophils to sites of inflammation and infection and signals monocytes to increase their expression of the firm adhesion molecule β2 integrin . High levels of IL-8 are detected in the serum of post-MI patients or patients with high cholesterol and unstable angina [50, 51]. IL-8 is also present in human atherosclerotic plaques, where it contributes to plaque instability by promoting matrix degradation . IL-8 is thus a critical instigator of plaque rupture [51, 52]. Induction of IL-8 transcription is BET-dependent. Apabetalone displaced BRD4 from the promoter of IL-8, where it accumulates following TNFα stimulation (Fig. 3e). Apabetalone’s epigenetic regulation of IL-8 transcription likely contributes to decreases in firm adhesion and plaque rupture [22, 53].
Macrophage differentiation, plaque development, and rupture
Firm adhesion enables monocyte transmigration through the endothelium. As monocytes arrive in the intima [25, 54], they differentiate into pro-inflammatory MI macrophages in response to cytokines and growth factors  (Fig. 1). CSF-2 (GM-CSF) is a prominent differentiation inducing cytokine/growth factor , whose expression is downregulated by apabetalone. IPA® predicted that CSF-2 signaling activity was inhibited in ASSURE CVD patient plasma by apabetalone (Table 7). This is expected to impede monocyte to M1 macrophage differentiation. In response to stimulation, macrophages are activated, which upregulates scavenger receptor expression. This enables the macrophages to internalize oxLDL and causes them to become lipid-laden foam cells (Fig. 1). Foam cells in the intima are a hallmark of early atherosclerosis [3, 54]. Through its regulation of inflammatory gene expression (CSF-2, MCP-1, IL-1β, C-X-C motif chemokine 10 (CXCL10), interleukin-15 (IL-15), and IL-6 (Tables 1 and 2), apabetalone should interfere with the differentiation of monocytes to M1 macrophages to foam cells and, thus, plaque development.
Atherosclerotic plaque development is the combined consequence of chronic inflammation , environmental stresses (ROS, hypoxia), plaque structure (extracellular matrix, collagen, lipids), and evolving biological processes (infiltrating immune cells, apoptosis) . Serious problems arise when the plaque ruptures, causing 67% of all fatal MIs and sudden cardiac deaths . Matrix metalloproteinases (MMPs) are the modelers and remodelers of the plaque’s extracellular matrix, and as their abundance increases, the plaque’s stability is undermined . TLR2 signaling directly induces MMP expression through MYD88 and NF-κB activation , while IL-8 indirectly regulates MMP abundance. The pan-BETi JQ1 decreased MMP expression and activity in HUVECs, mouse macrophages, and ECV304, an endothelial-like cell line . BD2-selective apabetalone inhibits IL-8, TLR2, and endothelial cell expression of multiple plaque-destabilizing genes (Tables 1 and 2). The abundance of key plaque destabilizers (MMP-3, MMP-12, and pappalysin 1 (PAPPA) was substantially lower in the plasma of ASSURE CVD patients with apabetalone treatment (vs placebo, Table 8). Importantly, plaque vulnerability (plaque length, arc, and index) and MACE events also decreased with apabetalone treatment . Animal studies had previously indicated that BETi affect plaque parameters; JQ1 attenuated angiotensin II-induced abdominal aortic aneurysm in ApoE (−/−) mice , and apabetalone reduced atherosclerosis in hyperlipidemic ApoE-deficient mice . Thus, our data combined with previous studies strongly suggest that apabetalone may inhibit plaque development and promote plaque stability through its epigenetic regulation of transcription.
Atherosclerosis is no longer defined solely as a lipid deposition disease. The CANTOS trial was the first phase III trial directly targeting inflammation as a CVD therapeutic strategy, and this novel approach resulted in MACE reduction . Inflammation, however, is a critical form of cellular communication and is required to generate a defensive immune response. Blunted cytokine responses have the potential to increase the rate of infections and infestations; canakinumab did increase the incidence of fatal infections in patients by nearly two fold (0.31 vs. 0.18 per 100 person-years, p = 0.02) . In contrast, apabetalone treatment, with its capacity to regulate multiple inflammatory factors (including cytokines, adhesion molecules, and APR proteins), does not impact the rate of infections or infestations in patients (safety data from phase II ASSURE, ASSERT, SUSTAIN, and ongoing phase III BETonMACE clinical trials) ([60, 61] data not shown). Apabetalone, therefore, is a CVD therapeutic candidate that effectively targets inflammation while maintaining a safety profile necessary for extended treatment.
Our in vitro work directly supports key findings of our clinical data: apabetalone, a BD2-selective BETi, downregulates the expression of multiple VI and atherogenic factors. Mechanistically, inflammation-driven gene expression requires direct BET protein interactions with chromatin and transcription factors, and apabetalone is capable of preventing BRD4 associations with key enhancers and promoters. Consequently, gene transcripts encoding proteins with roles in monocyte recruitment, leukocyte capture, rolling, adhesion, firm adhesion, macrophage differentiation, plaque development and stability are all downregulated by apabetalone (Fig. 1). The reduction in VI and atherogenic factors in CVD patient plasma correlates with the reduction in both MACE  and corresponding plaque parameters . Apabetalone is at the front line of the new paradigm shift of targeting inflammation in atherosclerosis. Epigenetic inhibition of BET-dependent inflammatory gene expression by apabetalone is anticipated to contribute to the prevention of MACE in the ongoing study BETonMACE.
All cells were incubated at 37 °C in humidified atmosphere enriched with 5% CO2.
Pooled HUVECs (Lonza CC-2519, LOT 0000636877 and 0000475053) were expanded in Endothelial Cell Growth Base Media (R&D Systems CCM027) with Endothelial Growth Supplement, 1× Penicillin-Streptomycin (Gibco, Thermo Fisher), and 5ug/mL Plasmocin (invivo Gen). Cells were expanded until passage 3 or 4 (p3 or p4) only and immediately used in experiments.
HAECs (Lonza CC-2535, Lot 0000337673) were expanded in EGM-2 media (Lonza CC-3162) until passage 5, frozen (1 T75 per vial), and stored in liquid nitrogen. One vial was thawed into 4 T75 and expanded until 80% confluency (6–7 days).
THP-1 monocytes (Sigma or ATCC) were subcultured in RPMI-1640 media (Gibco/Life Technologies 11875-093) supplemented with 10% heat-inactivated FBS (Gibco 12483-020 Canada origin), 1× Penicillin-Streptomycin (Gibco, Thermo Fisher), 5ug/mL Plasmocin (invivo Gen), 1 mM sodium pyruvate (Gibco 11360-070), 10 mM HEPES pH 7.4 (Millipore TMS-003-C), and 0.05 mM beta-mercaptoethanol (Sigma M6250).
Nuclear translocation of RelA
HUVECs were treated with apabetalone (5 or 20 μM) or DMSO and TNFα (10 ng/ml) for 2 h. Nuclear and cytoplasmic lysates were prepared using NE-PER kit (ThermoScientific, 78833) with freshly added protease inhibitor cocktail (BioShop or Sigma-Aldrich), phosSTOP phosphatase inhibitor (Roche 04906837001), and 0.5uM TSA (HDAC inhibitor). Protein concentration was determined with BioRad DC assay and lysate was added to NuPAGE LDS sample buffer (Novex/Invitrogen/Life Technologies NP0007) and 20 ug of total protein was loaded onto a NuPAGE 4-12% Bis-Tris gel (Novex/Invitrogen/Life Technologies NP0321BOX). For immunoblotting, the following primary antibodies were used: anti-p65 (Abcam, ab16502), anti-phospho p65 S536 (Cell Signaling, 3033), anti-BRD2 (Bethyl, A302-583A), anti-alpha tubulin (Sigma, SAB3500023), and anti-β-actin conjugated to peroxidase (Sigma, A3854). Secondary antibodies used were goat anti-rabbit IgG H&L chain specific peroxidase (Calbiochem, 401353) and rabbit anti-chicken IgY H&L chain specific peroxidase (Abcam, ab6753). Immunoreactive proteins were visualized by the chemiluminescent reagent ECLTM prime (GE Healthcare, RPN2232).
PROTAC MZ-1 knock-down of BET proteins
HUVECs or THP-1 cells were pretreated with apabetalone (5 or 20 μM), MZ-1 (0.5 μM or 1 μM; Tocris #6154), or vehicle (DMSO) for 4 h. They were then stimulated with TNFα (10 ng/ml) in the presence of apabetalone, MZ-1, or DMSO for 2 h before lysates were harvested. mRNA was harvested using Catcher PLUS kits according to the manufacturer’s instructions (Life Technologies). Protein lysis buffer consisted of PBS (pH 7.4, Life Technologies) supplemented with 1% Nonidet® P40, 1% SDS, 0.5% sodium deoxycholate, 60 mM sodium fluoride, 1 mM sodium orthovanadate, 5 mM sodium pyrophosphate and freshly added protease inhibitor cocktail (BioShop or Sigma-Aldrich), phosSTOP phosphatase inhibitor (Roche 04906837001), and 0.5 μM trichostatin A (HDAC inhibitor). Lysates were sonicated at 75% output for 15 seconds with a Branson SLPt sonicator (Branson Ultrasonics, Danbury, CT). Insoluble material was removed by centrifugation at 10,000g at 4 °C for 3 min. The supernatant was removed and stored at − 80 °C until use. Protein concentration was determined with BioRad DC assay and lysate was added to NuPAGE LDS sample buffer (Novex/Invitrogen/Life Technologies NP0007) and 20 μg of total protein was loaded onto a NuPAGE 4-12% Bis-Tris gel (Novex/Invitrogen/Life Technologies NP0321BOX). For immunoblotting, the following primary antibodies were used: anti-BRD2 (Bethyl, A700-008), anti-BRD3 (Bethyl, A302-368A), anti-BRD4 (Bethyl, A700-005), anti-p65 (Abcam, ab16502), anti-phospho p65 S536 (Cell Signaling, 3033), and anti-β-actin conjugated to peroxidase (Sigma, A3854). Secondary antibody used was goat anti-rabbit IgG H&L chain specific peroxidase (Calbiochem, 401353). Immunoreactive proteins were visualized by the chemiluminescent reagent ECLTM prime (GE Healthcare, RPN2232).
Cell pellets (~ 20–30 million cells) were prepared from p3 HUVECs pretreated with apabetalone (5 or 20 μM) or vehicle (DMSO) for 1 h then stimulated with addition of TNFα (10 ng/ml) for 1 h. Cells were crosslinked with 1% formaldehyde, quenched with 125 mM Glycine, and washed pellets were shipped on dry ice to Active Motif (Carlsbad, CA) who prepared chromatin from the lysates, performed ChIP reactions and qPCR, and performed basic data analysis.
mRNA was isolated from THP-1 cells and HUVEC cells, pretreated with apabetalone (5 or 20 uM) or vehicle (DMSO) for 1 h before stimulation with TNFα (10 ng/ml) in the presence of apabetalone or DMSO for 1 h (Additional file 1: Figure S1) or 4 h (all other experiments) (Catcher PLUS kits; Life Technologies). Taqman PCR assays were obtained from Applied Biosystems/Life Technologies. Real-time PCR was used to determine the abundance of the transcript relative to the endogenous control cyclophilin in the same sample using the RNA Ultrasense One-step qRT-PCR kit (Life Technologies). Data was acquired using a ViiA-7 Real-Time PCR apparatus (Applied Biosystems). Analysis was performed as 2^ (CT cyclophilin – CT marker) and results were normalized to DMSO treated samples.
HUVECs were pretreated with apabetalone (5 or 20 μM) or vehicle (DMSO) for 1 h before addition of TNFα (10 ng/ml) for 4 h. HUVEC total RNA was then isolated (RNEasy isolation kit, Qiagen) and sent to NanoString for multiplex gene expression analysis (255 human genes) with the nCounter® Inflammation v2 Panel. NanoString was run by the University of Alberta pathology core and data was analyzed in house with the nSolverTM software and IngenuityR Pathway Analysis software (Oct 2018 update). Genes with fold change > 1.3 and <− 1.3 were used in IngenuityR Pathway Analysis.
Flow cytometric analysis of VCAM-1 and SELE HUVEC surface expression and MCP-1 secretion
HUVECs were stimulated for 4 h with DMSO or TNFα ± apabetalone (5 or 20 μM). Surface expression of VCAM-1 and SELE was labeled with FITC conjugated anti-CD106 and APC conjugated anti-CD62E (BD Bioscience) and quantified by flow cytometry. Mean fluorescence intensity (MFI) relative to the unstimulated DMSO control were reported. HUVECs were stimulated for overnight with DMSO or TNFα ± apabetalone (5 or 20 μM). Supernatant was collected and MCP-1 secretion was measured by a cytometric bead array (MCP-1 flex set, BD Bioscience), and detected by flow cytometry.
Static adhesion assay
HUVECs were seeded into black/clear bottom 96-well plates (Thermo Scientific™ Nunc™ MicroWell™ 96-Well Optical-Bottom Plates with Polymer Base, Thermo Scientific cat #165305) at a density of 12,500 cells/well. Twenty-four hours after seeding, cells were treated as dep. An initial 1-h pre-conditioning was followed by 4 h 2.5 ng/mL TNFα (Peprotech cat #300-01A-50UG, Lot 0607B25 G2516) treatment (in presence of compound or DMSO). THP-1 cells were stained with 5 μM calcein-AM (Thermo Fisher Scientific cat # C3100MP) in serum-free RPMI-1640 media at a density of 2.5 × 106 cells/ml for 30 min at 37 °C, 5% CO2 and washed twice in THP-1 media. Endothelial cells were washed once in THP-1 media before addition of 200 μl/well of calcein-AM labeled THP-1 at a density of 0.5 × 106 cells/ml for 1 h at 37 °C and 5% CO2. Unbound monocytes were removed by 4–6 washes (90° turn of plate between wash) with pre-warmed THP-1 media. Once all unbound THP-1 cells were removed, plates were washed 2× with PBS, fixed in 4% paraformaldehyde for 5 min, and washed 2× with PBS. The amount of bound monocytes was indirectly determined by measuring the fluorescent signal on a plate reader (SpectraMax M2, Molecular Devices). A 9-point well scan was performed at an excitation of 485 nm and emission of 520 nm. Additionally, representative images were captured on an Eclipse TS100 microscope (Nikon) with a × 10 objective and a Zyla sCMOS camera (Andor).
Flow adhesion assay
HAECs were seeded onto gelatin-coated standard glass microscope slides at a density of 0.2 × 106 cells/slide and treated according to the outlined regimen (Fig. 5b). Following treatment, HAECs were mounted in the flow chamber and placed on an inverted Eclipse TS100 microscope (Nikon) with a × 10 objective and a Zyla sCMOS camera (Andor). A heat lamp maintained the temperature at approximately 37 °C. Flow chambers are composed of a 0.01-in.-thick silicone rubber gaskets with a removed rectangular section to form the flow channel (0.5 × 1.97 in.) and a plexiglass top plate providing the inlet and outlet as described in Viegas (). THP-1 cells were perfused through the flow chamber in full THP-1 media at a density of 0.4 × 106 cells/ml using a 10 cc syringe mounted on a syringe pump (KDS 200, dual syringe infusion pump, KD Scientific) according to the following scheme:
• 3 min at 50 s−1
• 3 min at 25 s−1
• 120 s−1 to take pictures
A 2-min video was captured at 50 and 25 s−1 shear rate and 10 images taken at a high shear rate of 120 s−1 where all unbound THP-1 are removed. Monocyte adhesion was quantified in ImageJ using the “Find Maxima” function.
SOMAScanTM Proteomic analysis
The ASSURE study (NCT01067820) design and rationale has been published previously . Briefly, it was a phase II, placebo-controlled, multi-center, double-blind study. The study was conducted in accordance with the ethical standards of the responsible committee on human experimentation (institutional and national) and with the Helsinki Declaration of 1975, as revised in 2000. Informed consent was obtained from all study participants. Participants all had unstable CAD, with at least one > 20% lumen stenosis in a native epicardial coronary artery on visual estimation of a clinically indicated coronary angiogram. Patients received placebo or 100 mg apabetalone twice per day. All patients also received standard medical therapy, either atorvastatin (10, 20, or 40 mg) or rosuvastatin (5, 10, or 20 mg). Baseline and end-of-study (26 weeks) plasma samples (47 placebo and 47 apabetalone treated) from ASSURE were analyzed using the SOMAScanTM 1.3 K proteomic technology (Somalogic Inc., Boulder, CO). The abundance of 1305 proteins was assessed. Wilcoxon signed-rank tests were run versus baseline. Mann-Whitney U test were run to compare median change and percent change between apabetalone treated patients and placebo. IPA® software analyzed changes (> 10%, p < 0.05) in proteins affected by apabetalone treatment (versus placebo) and predicted its impact on canonical pathways, upstream regulators, and diseases and biological functions.
Availability of data and materials
The datasets generated and/or analyzed during the current study are not publicly available. Reasonable requests for data will be considered. All genes, proteins, pathways, upstream regulators, and diseases and biological functions discussed are provided in the Tables within the paper itself.
- ApoE (−/−):
Serum amyloid P-component
ApoA-I Synthesis Stimulation and Intravascular Ultrasound for Coronary Atheroma Regression Evaluation
Bromodomain and extraterminal protein
Bromodomain and extraterminal protein inhibitor
Bromodomain containing 2
Bromodomain containing 3
Bromodomain containing 4
Canakinumab Anti-Inflammatory Thrombosis Outcomes Study
C-C motif chemokine receptor 1
C-C motif chemokine receptor 2
Cluster of differentiation 106 (VCAM-1)
Cluster of differentiation 40 ligand
Cluster of differentiation 44
Cluster of differentiation 62E (SELE)
Complement factor b
- CO2 :
Granulocyte-macrophage colony stimulating factor
C-X3-C motif chemokine ligand 1
C-X-C motif chemokine 10
C-X-C motif chemokine ligand 3
Endothelial cell growth medium-2
Fetal bovine serum
Human aortic endothelial cell
Hepatocyte growth factor
High mobility group box 1
- HMG-CoA :
Human umbilical vein endothelial cell
Interleukin 1 alpha
Interleukin 1 beta
Interleukin 1 receptor
Interferon-induced protein with tetratricopeptide repeats 2
Ingenuity pathway analysis
Interferon regulatory factor 1
Jun N-terminal kinase
- LDLR (−/−):
Major adverse cardiac events
Monocyte chemoattractant protein 1
Macrophage inhibitory factor
Matrix metalloproteinase 3
Matrix metalloproteinase 12
Messenger ribonucleic acid
Innate immune signal transduction adaptor
Nuclear factor kappa-light-chain-enhancer of activated B cells
Polymerase chain reaction
Proteolysis targeting chimeric molecule
Positive transcription elongation factor
RELA proto-oncogene, NF-KB Subunit
RELB proto-oncogene, NF-KB Subunit
Reactive oxygen species
Roswell Park Memorial Institute-1640
Stress-activated protein kinase
Type 2 diabetes mellitus
Transforming growth factor beta 3
Toll-like receptor adaptor molecule 1
Toll-like receptor 2
Toll-like receptor 3
Toll-like receptor 4
- TLR4 LY96:
Toll-like receptor 4:lymphocyte antigen 96 complex
TNF alpha-induced protein 3
Tumor necrosis factor alpha
Tumor necrosis factor receptor
TNF receptor superfamily member 11b
TNFRSF1A associated via death domain
Triggering receptor expressed on myeloid cells 1
Vascular cell adhesion molecule 1
Very late antigen-4
Mestas J, Ley K. Monocyte-endothelial cell interactions in the development of atherosclerosis. Trends Cardiovasc Med. 2008;18:228–32. https://doi.org/10.1016/j.tcm.2008.11.004.
Tajbakhsh A, Rezaee M, Kovanen PT, Sahebkar A. Efferocytosis in atherosclerotic lesions: Malfunctioning regulatory pathways and control mechanisms. Pharmacol Ther. 2018;188:12–25. https://doi.org/10.1016/j.pharmthera.2018.02.003.
Chistiakov DA, Melnichenko AA, Myasoedova VA, Grechko AV, Orekhov AN. Mechanisms of foam cell formation in atherosclerosis. J Mol Med (Berl). 2017;95:1153–65. https://doi.org/10.1007/s00109-017-1575-8.
Stefanadis C, Antoniou CK, Tsiachris D, Pietri P. Coronary atherosclerotic vulnerable plaque: current perspectives. J Am Heart Assoc. 2017;6. https://doi.org/10.1161/JAHA.117.005543.
World Heath Organization. Cardiovascular diseases (CVDs) [Webpage]. 2017. https://www.who.int/en/news-room/fact-sheets/detail/cardiovascular-diseases-(cvds). [updated May 17, 2017; cited 2019 January 10, 2019].
Huang B, Yang XD, Zhou MM, Ozato K, Chen LF. Brd4 coactivates transcriptional activation of NF-kappaB via specific binding to acetylated RelA. Mol Cell Biol. 2009;29:1375–87. https://doi.org/10.1128/MCB.01365-08.
Itzen F, Greifenberg AK, Bosken CA, Geyer M. Brd4 activates P-TEFb for RNA polymerase II CTD phosphorylation. Nucleic Acids Res. 2014;42:7577–90. https://doi.org/10.1093/nar/gku449.
Nicodeme E, Jeffrey KL, Schaefer U, Beinke S, Dewell S, Chung CW, et al. Suppression of inflammation by a synthetic histone mimic. Nature. 2010;468:1119–23. https://doi.org/10.1038/nature09589.
Prinjha RK, Witherington J, Lee K. Place your BETs: the therapeutic potential of bromodomains. Trends Pharmacol Sci. 2012;33:146–53. https://doi.org/10.1016/j.tips.2011.12.002.
Pierce JW, Lenardo M, Baltimore D. Oligonucleotide that binds nuclear factor NF-kappa B acts as a lymphoid-specific and inducible enhancer element. Proc Natl Acad Sci U S A. 1988;85:1482–6. https://www.ncbi.nlm.nih.gov/pubmed/3125549.
Baltimore D. NF-kappaB is 25. Nat Immunol. 2011;12:683–5. https://doi.org/10.1038/ni.2072.
Chen LF, Williams SA, Mu Y, Nakano H, Duerr JM, Buckbinder L, et al. NF-kappaB RelA phosphorylation regulates RelA acetylation. Mol Cell Biol. 2005;25:7966–75. https://doi.org/10.1128/MCB.25.18.7966-7975.2005.
Brown JD, Lin CY, Duan Q, Griffin G, Federation A, Paranal RM, et al. NF-kappaB directs dynamic super enhancer formation in inflammation and atherogenesis. Mol Cell. 2014;56:219–31. https://doi.org/10.1016/j.molcel.2014.08.024.
Das S, Senapati P, Chen Z, Reddy MA, Ganguly R, Lanting L, et al. Regulation of angiotensin II actions by enhancers and super-enhancers in vascular smooth muscle cells. Nat Commun. 2017;8:1467. https://doi.org/10.1038/s41467-017-01629-7.
Filippakopoulos P, Knapp S. The bromodomain interaction module. FEBS Lett. 2012;586:2692–704. https://doi.org/10.1016/j.febslet.2012.04.045.
Jang MK, Mochizuki K, Zhou M, Jeong HS, Brady JN, Ozato K. The bromodomain protein Brd4 is a positive regulatory component of P-TEFb and stimulates RNA polymerase II-dependent transcription. Mol Cell. 2005;19:523–34. https://doi.org/10.1016/j.molcel.2005.06.027.
LeRoy G, Rickards B, Flint SJ. The double bromodomain proteins Brd2 and Brd3 couple histone acetylation to transcription. Mol Cell. 2008;30:51–60. https://doi.org/10.1016/j.molcel.2008.01.018.
Doroshow DB, Eder JP, LoRusso PM. BET inhibitors: a novel epigenetic approach. Ann Oncol. 2017;28:1776–87. https://doi.org/10.1093/annonc/mdx157.
Picaud S, Wells C, Felletar I, Brotherton D, Martin S, Savitsky P, et al. RVX-208, an inhibitor of BET transcriptional regulators with selectivity for the second bromodomain. Proc Natl Acad Sci U S A. 2013;110:19754–9. https://doi.org/10.1073/pnas.1310658110.
McLure KG, Gesner EM, Tsujikawa L, Kharenko OA, Attwell S, Campeau E, et al. RVX-208, an inducer of ApoA-I in humans, is a BET bromodomain antagonist. PLoS One. 2013;8:e83190. https://doi.org/10.1371/journal.pone.0083190.
Nicholls SJ, Gordon A, Johansson J, Wolski K, Ballantyne CM, Kastelein JJ, et al. Efficacy and safety of a novel oral inducer of apolipoprotein a-I synthesis in statin-treated patients with stable coronary artery disease. a randomized controlled trial. J Am Coll Cardiol. 2011;57:1111–9. https://doi.org/10.1016/j.jacc.2010.11.015.
Shishikura D, Kataoka Y, Honda S, Takata K, Kim SW, Andrews J, et al. The effect of bromodomain and extra-terminal inhibitor apabetalone on attenuated coronary atherosclerotic plaque: insights from the ASSURE trial. Am J Cardiovasc Drugs. 2018. https://doi.org/10.1007/s40256-018-0298-8.
Jahagirdar R, Zhang H, Azhar S, Tobin J, Attwell S, Yu R, et al. A novel BET bromodomain inhibitor, RVX-208, shows reduction of atherosclerosis in hyperlipidemic ApoE deficient mice. Atherosclerosis. 2014;236:91–100. https://doi.org/10.1016/j.atherosclerosis.2014.06.008.
Zengerle M, Chan KH, Ciulli A. Selective small molecule induced degradation of the BET bromodomain protein BRD4. ACS Chem Biol. 2015;10:1770–7. https://doi.org/10.1021/acschembio.5b00216.
Ley K, Laudanna C, Cybulsky MI, Nourshargh S. Getting to the site of inflammation: the leukocyte adhesion cascade updated. Nat Rev Immunol. 2007;7:678–89. https://doi.org/10.1038/nri2156.
Abdolmaleki F, Gheibi Hayat SM, Bianconi V, Johnston TP, Sahebkar A. Atherosclerosis and immunity: a perspective. Trends Cardiovasc Med. 2018. S1050-1738(18)30225-1 [pii] https://doi.org/10.1016/j.tcm.2018.09.017.
Nicholls SJ, Puri R, Wolski K, Ballantyne CM, Barter PJ, Brewer HB, et al. Effect of the BET protein inhibitor, RVX-208, on progression of coronary atherosclerosis: results of the phase 2b, randomized, double-blind, multicenter, ASSURE trial. Am J Cardiovasc Drugs. 2016;16:55–65. https://doi.org/10.1007/s40256-015-0146-z.
Huang M, Zeng S, Zou Y, Shi M, Qiu Q, Xiao Y, et al. The suppression of bromodomain and extra-terminal domain inhibits vascular inflammation by blocking NF-kappaB and MAPK activation. Br J Pharmacol. 2017;174:101–15. https://doi.org/10.1111/bph.13657.
Leon BM, Maddox TM. Diabetes and cardiovascular disease: epidemiology, biological mechanisms, treatment recommendations and future research. World J Diabetes. 2015;6:1246–58. https://doi.org/10.4239/wjd.v6.i13.1246.
Pirillo A, Norata GD, Catapano AL. LOX-1, OxLDL, and atherosclerosis. Mediators Inflamm. 2013;2013:152786. https://doi.org/10.1155/2013/152786.
Charo IF, Taub R. Anti-inflammatory therapeutics for the treatment of atherosclerosis. Nat Rev Drug Discov. 2011;10:365–76. https://doi.org/10.1038/nrd3444.
Ridker PM. How common is residual inflammatory risk? Circulation Research. 2017;120:617–9. https://doi.org/10.1161/CIRCRESAHA.116.310527.
Aday AW, Ridker PM. Antiinflammatory therapy in clinical care: the CANTOS trial and beyond. Front Cardiovasc Med. 2018;5:62. https://doi.org/10.3389/fcvm.2018.00062.
Gimbrone MA Jr, Garcia-Cardena G. Endothelial Cell dysfunction and the pathobiology of atherosclerosis. Circ Res. 2016;118:620–36. https://doi.org/10.1161/CIRCRESAHA.115.306301.
Deshmane SL, Kremlev S, Amini S, Sawaya BE. Monocyte chemoattractant protein-1 (MCP-1): an overview. J Interferon Cytokine Res. 2009;29:313–26. https://doi.org/10.1089/jir.2008.0027.
Ramji DP, Davies TS. Cytokines in atherosclerosis: key players in all stages of disease and promising therapeutic targets. Cytokine Growth Factor Rev. 2015;26:673–85. https://doi.org/10.1016/j.cytogfr.2015.04.003.
McEver RP. Selectins: initiators of leucocyte adhesion and signalling at the vascular wall. Cardiovasc Res. 2015;107:331–9. https://doi.org/10.1093/cvr/cvv154.
Marshall BT, Long M, Piper JW, Yago T, McEver RP, Zhu C. Direct observation of catch bonds involving cell-adhesion molecules. Nature. 2003;423:190–3. https://doi.org/10.1038/nature01605.
Čejková S, Králová-Lesná I, Poledne R. Monocyte adhesion to the endothelium is an initial stage of atherosclerosis development. Cor et Vasa. 2016;58:e419–e25 https://doi.org/10.1016/j.crvasa.2015.08.002.
Davies MJ, Gordon JL, Gearing AJ, Pigott R, Woolf N, Katz D, et al. The expression of the adhesion molecules ICAM-1, VCAM-1, PECAM, and E-selectin in human atherosclerosis. J Pathol. 1993;171:223–9. https://doi.org/10.1002/path.1711710311.
Cybulsky MI, Iiyama K, Li H, Zhu S, Chen M, Iiyama M, et al. A major role for VCAM-1, but not ICAM-1, in early atherosclerosis. J Clin Invest. 2001;107:1255–62. https://doi.org/10.1172/JCI11871.
Muller WA. Getting leukocytes to the site of inflammation. Vet Pathol. 2013;50:7–22. https://doi.org/10.1177/0300985812469883.
Barreiro O, Vicente-Manzanares M, Urzainqui A, Yanez-Mo M, Sanchez-Madrid F. Interactive protrusive structures during leukocyte adhesion and transendothelial migration. Front Biosci. 2004;9:1849–63. https://www.ncbi.nlm.nih.gov/pubmed/14977592.
Shen B, Delaney MK, Du X. Inside-out, outside-in, and inside-outside-in: G protein signaling in integrin-mediated cell adhesion, spreading, and retraction. Curr Opin Cell Biol. 2012;24:600–6. https://doi.org/10.1016/j.ceb.2012.08.011.
Cerutti C, Ridley AJ. Endothelial cell-cell adhesion and signaling. Exp Cell Res. 2017;358:31–8. https://doi.org/10.1016/j.yexcr.2017.06.003.
Park JG, Ryu SY, Jung IH, Lee YH, Kang KJ, Lee MR, et al. Evaluation of VCAM-1 antibodies as therapeutic agent for atherosclerosis in apolipoprotein E-deficient mice. Atherosclerosis. 2013;226:356–63. https://doi.org/10.1016/j.atherosclerosis.2012.11.029.
De Caterina R, Basta G, Lazzerini G, Dell’Omo G, Petrucci R, Morale M, et al. Soluble vascular cell adhesion molecule-1 as a biohumoral correlate of atherosclerosis. Arterioscler Thromb Vasc Biol. 1997;17:2646–54. https://www.ncbi.nlm.nih.gov/pubmed/9409238.
Lubrano V, Balzan S. Consolidated and emerging inflammatory markers in coronary artery disease. World J Exp Med. 2015;5:21–32. https://doi.org/10.5493/wjem.v5.i1.21.
Gerszten RE, Garcia-Zepeda EA, Lim YC, Yoshida M, Ding HA, Gimbrone MA Jr, et al. MCP-1 and IL-8 trigger firm adhesion of monocytes to vascular endothelium under flow conditions. Nature. 1999;398:718–23. https://doi.org/10.1038/19546.
Velasquez IM, Frumento P, Johansson K, Berglund A, de Faire U, Leander K, et al. Association of interleukin 8 with myocardial infarction: results from the Stockholm Heart Epidemiology Program. Int J Cardiol. 2014;172:173–8. https://doi.org/10.1016/j.ijcard.2013.12.170.
Autieri MV. Pro- and anti-inflammatory cytokine networks in atherosclerosis. International Scholarly Research Network ISRN Vascular Medicine. 2012;2012:17. https://doi.org/10.5402/2012/987629.
Apostolakis S, Vogiatzi K, Amanatidou V, Spandidos DA. Interleukin 8 and cardiovascular disease. Cardiovasc Res. 2009;84:353–60. https://doi.org/10.1093/cvr/cvp241.
Nicholls SJ, Ray KK, Johansson JO, Gordon A, Sweeney M, Halliday C, et al. Selective BET protein inhibition with apabetalone and cardiovascular events: a pooled analysis of trials in patients with coronary artery disease. Am J Cardiovasc Drugs. 2018;18:109–15. https://doi.org/10.1007/s40256-017-0250-3.
Wang D, Wang Z, Zhang L, Wang Y. Roles of cells from the arterial vessel wall in atherosclerosis. Mediators Inflamm. 2017;2017:8135934. https://doi.org/10.1155/2017/8135934.
Ushach I, Zlotnik A. Biological role of granulocyte macrophage colony-stimulating factor (GM-CSF) and macrophage colony-stimulating factor (M-CSF) on cells of the myeloid lineage. J Leukoc Biol. 2016;100:481–9. https://doi.org/10.1189/jlb.3RU0316-144R.
Tatsumi K, Mackman N. Tissue factor and atherothrombosis. J Atheroscler Thromb. 2015;22:543–9. https://doi.org/10.5551/jat.30940.
Galis ZS, Khatri JJ. Matrix metalloproteinases in vascular remodeling and atherogenesis: the good, the bad, and the ugly. Circ Res. 2002;90:251–62. https://www.ncbi.nlm.nih.gov/pubmed/11861412.
Falck-Hansen M, Kassiteridi C, Monaco C. Toll-like receptors in atherosclerosis. Int J Mol Sci. 2013;14:14008–23. https://doi.org/10.3390/ijms140714008.
Duan Q, Mao X, Liao C, Zhou H, Sun Z, Deng X, et al. Inhibition of BET bromodomain attenuates angiotensin II induced abdominal aortic aneurysm in ApoE(-/-) mice. Int J Cardiol. 2016;223:428–32. https://doi.org/10.1016/j.ijcard.2016.08.238.
Wasiak S, Gilham D, Tsujikawa LM, Halliday C, Calosing C, Jahagirdar R, et al. Downregulation of the complement cascade in vitro, in mice and in patients with cardiovascular disease by the BET protein inhibitor apabetalone (RVX-208). J Cardiovasc Transl Res. 2017;10:337–47. https://doi.org/10.1007/s12265-017-9755-z.
Kulikowski E, Halliday C, Johansson J, Sweeney M, Lebioda K, Wong N, et al. Apabetalone mediated epigenetic modulation is associated with favorable kidney function and alkaline phosphatase profile in patients with chronic kidney disease. Kidney Blood Press Res. 2018;43:449–57. https://doi.org/10.1159/000488257.
Viegas KD, Dol SS, Salek MM, Shepherd RD, Martinuzzi RM, Rinker KD. Methicillin resistant Staphylococcus aureus adhesion to human umbilical vein endothelial cells demonstrates wall shear stress dependent behaviour. Biomed Eng Online. 2011;10:20. https://doi.org/10.1186/1475-925X-10-20.
Nicholls SJ, Gordon A, Johannson J, Ballantyne CM, Barter PJ, Brewer HB, et al. ApoA-I induction as a potential cardioprotective strategy: rationale for the SUSTAIN and ASSURE studies. Cardiovasc Drugs Ther. 2012;26:181–7. https://doi.org/10.1007/s10557-012-6373-5.
This work was privately funded by Resverlogix.
Ethics approval and consent to participate
The ASSURE study (NCT01067820) design and rationale has been published previously . Briefly, it was a phase II, placebo-controlled, multi-center, double-blind study. The study was conducted in accordance with the ethical standards of the responsible committee on human experimentation (institutional and national) and with the Helsinki Declaration of 1975, as revised in 2000. Informed consent was obtained from all study participants.
Consent for publication
All authors that are Resverlogix employees receive salaries and shares from the company.
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Figure S1. Overall abundance of BRD4 protein levels in HUVECs did not change with apabetalone treatment (western blot). HUVEC cells were co-treated with TNFα and either apabetalone, RVX compound B, or MZ-1 (0.2uM) for 24hrs. Western blot of protein lysates was probed with anti-BRD4 antibody (Bethyl, A700-005) and goat anti-rabbit IgG H&L chain specific peroxidase (Calbiochem, 401353). Anti-β actin conjugated to peroxidase (Sigma, A3854) was used as a loading control. Figure S2. In HUVECs, 1 hour apabetalone pretreatment significantly inhibited TNFα-induced expression of MCP-1, SELE, and VCAM-1 (1 hour stimulation). Cells treated in parallel were processed for ChIP or RT-PCR according to the protocols found in Methods. Statistical significance was determined through 1-way ANOVA analysis followed by Tukey's Multiple Comparison Test, where ***p<0.001 (PPTX 203 kb)
About this article
- THP-1 monocytes
- Vascular inflammation