Carbenoxolone Blocks Endotoxin-Induced Protein Kinase R (PKR) Activation and High Mobility Group Box 1 (HMGB1) Release
- 24 Downloads
The pathogen- and damage-associated molecular patterns (for example, bacterial endotoxin and adenosine 5′-triphosphate (ATP)) activate the double-stranded RNA-activated protein kinase R (PKR) to trigger the inflammasome-dependent high mobility group box 1 (HMGB1) release. Extracellular ATP contributes to the inflammasome activation through binding to the plasma membrane purinergic P2X7 receptor (P2X7R), triggering the opening of P2X7R channels and the pannexin-1 (panx-1) hemichannels permeable for larger molecules up to 900 daltons. It was previously unknown whether panx-1 channel blockers can abrogate lipopolysaccharide (LPS)-induced PKR activation and HMGB1 release in innate immune cells. Here we demonstrated that a major gancao (licorice) component (glycyrrhizin, or glycyrrhizic acid) derivative, carbenoxolone (CBX), dose dependently abrogated LPS-induced HMGB1 release in macrophage cultures with an estimated IC50 ≈ 5 µmol/L. In an animal model of polymicrobial sepsis (induced by cecal ligation and puncture (CLP)), repetitive CBX administration beginning 24 h after CLP led to a significant reduction of circulating and peritoneal HMGB1 levels, and promoted a significant increase in animal survival rates. As did P2X7R antagonists (for example, oxidized ATP, oATP), CBX also effectively attenuated LPS-induced P2X7R/panx-1 channel activation (as judged by Lucifer Yellow dye uptake) and PKR phosphorylation in primary peritoneal macrophages. Collectively, these results suggested that CBX blocks LPS-induced HMGB1 release possibly through impairing PKR activation, supporting the involvement of PKR in the regulation of HMGB1 release.
Sepsis is an overwhelming systemic inflammatory response to severe infections, and remains the primary cause of mortality in medical intensive care units. It afflicts approximately 750,000 Americans each year, and costs the United States healthcare system nearly $17 billion annually (1). Current treatments are predominantly supportive and often ineffective, necessitating the continued search for effective therapies. The pathogenesis of sepsis is partly mediated by pathogen- and damage-associated molecular patterns (for example, endotoxins, adenosine 5′-triphosphate[ATP] or high mobility group box 1 [HMGB1]) (2), which activate innate immune cells via binding to various pattern-recognition receptors (for example, toll-like receptor 4 [TLR4], P2X7R, CD24, or Siglec-10) (3, 4, 5). For instance, crude endotoxins (containing trace amounts of bacterial proteins and nucleic acids) can stimulate macrophages to sequentially release early (for example, tumor necrosis factor [TNF], interleukin [IL]-1β and interferon [IFN]-γ) and late (for example, HMGB1) proinflammatory mediators (6,7). In animal models of endotoxemia or sepsis, circulating HMGB1 levels plateau between 24 and 36 hours (6,8), distinguishing HMGB1 from other early cytokines (9). Moreover, HMGB1-neutralizing antibodies confer protection against lethal endotoxemia (6) and sepsis (8,10) even when given 24 hours after the onset of sepsis, establishing HMGB1 as a late mediator of lethal inflammatory diseases (11).
The mechanisms underlying the regulation of endotoxin-induced HMGB1 release remain poorly elucidated. Emerging evidence has suggested an essential role for the inflammasome in the regulation of LPS/ATP-induced HMGB1 release (7,12), because genetic disruption of key inflammasome components (for example, caspase 1 or Nalp3) impaired the LPS/ATP-induced HMGB1 release. Recently, we discovered that the double-stranded RNA-activated protein kinase R (PKR) functions as the key regulator of inflammasome activation and HMGB1 release (7). It has been suggested that LPS activates the inflammasome signaling pathways partly through eliciting the passive ATP leakage (13). Indeed, ultrapure LPS (free from contaminating bacterial proteins and nucleic acids) fails to trigger HMGB1 release unless the initial LPS (10 µg/mL) priming is accompanied by a second stimulus (for example, ATP) (7,12). Similarly, ATP itself is unable to induce HMGB1 release without prior LPS exposure (12), although it can induce PKR phosphorylation (7) and inflammasome activation (14, 15, 16).
It has been suggested that ATP activates the inflammasome through binding to the purinergic P2X7 receptor (P2X7R) (5), which triggers an immediate (within milliseconds) opening of the ATP-gated P2X7R channel permeable for small cationic ions. Subsequently, the pannexin-1 (panx-1) hemichannels are recruited and activated, allowing passage of larger anionic molecules up to 900 Da (for example, ATP) (17, 18, 19). This feed-forwarding ATP-mediated ATP release contributes to the LPS-stimulated inflammasome activation (20) and subsequent inflammasome-dependent cytokine release (for example, IL-1β and IL-18) (14, 15, 16,21,22). It is not known whether agents capable of inhibiting the panx-1 hemichannel can inhibit LPS-induced PKR activation and HMGB1 release, thereby conferring protection against lethal sepsis.
Material and Methods
Bacterial endotoxin (lipopolysaccharide, LPS, E. coli 0111:B4), CBX (C4790), KN-62 (I2142), adenosine 5′-triphosphate-2′,3′-dialdehyde (oxidized ATP, oATP, A6779), brilliant blue G (BBG, B0770), Lucifer Yellow (L0144), paraformaldehyde (P6148) and mouse anti-β-actin antibodies (A1978) were obtained from Sigma-Aldrich (St. Louis, MO, USA). Calcein-AM (C3099), CM-DiI (C7001), Dulbecco’s modified Eagle medium (DMEM, 11995–065), penicillin/streptomycin (cat. 15140–122), fetal bovine serum (FBS, 26140079) and trypan blue (15250-061) were from Invitrogen/Life Technologies (Carlsbad, CA, USA). Anti-LC3 antibody (sc-16755), anti-PKR antibody (sc-6282), and HRP conjugated goat anti-mouse IgG (sc-2060) were from Santa Cruz Biotechnology Inc., Dallas, TX, USA. Anti-phosphorylated PKR antibody (07–886) was from Millipore (Billerica, MA, USA). HRP conjugated donkey anti-rabbit IgG was from GE Healthcare (NA934; Port Washington, NY, USA).
Murine macrophagelike RAW 264.7 cells were obtained from the American Type Culture Collection (ATCC, Rockville, MD, USA). Primary peritoneal macrophages were isolated from BALB/c mice (Taconic, Germantown, NY, USA; male, 7–8 wks, 20–25 g) at 2–3 d after intraperitoneal injection of 2 mL thioglycollate broth (4%) as described previously (35,36). Both RAW 264.7 cells and primary macrophages were cultured in DMEM supplemented with 1% penicillin/streptomycin and 10% FBS. Adherent macrophages were gently washed with, and cultured in, DMEM before stimulating with LPS (0.5 µg/mL) in the absence or presence of CBX or purinergic P2X7R antagonists (oATP, 50 µmol/L; BBG, 0.5 µmol/L; KN62, 0.5 µmol/L) for 16 h. Subsequently, the cell-conditioned culture media were analyzed for levels of HMGB1, nitric oxide (NO) and other cytokines by Western blotting analysis, the Griess reaction, ELISA, and cytokine antibodies arrays as described previously (36, 37, 38).
Cell Viability Assay
Cell viability was assessed by the trypan blue exclusion assay as described previously (39,40). Briefly, trypan blue was added to cell cultures at a final concentration of 0.08%. After incubation for 5 min at room temperature, the cell viability was assessed by the percentage of dyeexcluding cells in five 40x microscope fields.
The levels of HMGB1 in the culture medium, serum or peritoneal lavage fluid were determined by Western blotting analysis as described previously (6,41,42). The levels of total or phosphorylated PKR in primary macrophage cell lysates were determined by Western blotting analysis with reference to β-actin. Briefly, equal amounts of cellular proteins were resolved on sodium dodecyl sulfate (SDS)-polyacrylamide gels, and transferred to polyvinylidene difluoride (PVDF) membranes. After blocking with 5% nonfat milk, the membrane was incubated with respective antibodies (anti-PKR, 1:2000; anti-phospho-PKR, 1:1000; anti-β-actin. 1:5000) overnight. Subsequently, the membrane was incubated with the appropriate secondary antibody, and the immunoreactive bands were visualized by chemiluminescence technique.
The levels of TNF in the culture medium or serum were determined using commercial enzyme linked immunosorbent assay (ELISA) kits (MTA00, R&D Systems, Minneapolis, MN, USA) with reference to standard curves of purified recombinant TNF at various dilutions as described previously (37,38,42, 43, 44).
Nitric Oxide Assay
The levels of nitric oxide in the culture medium were determined indirectly by measuring the NO2-production with a colorimetric assay based on the Griess reaction (35,40). NO2- concentrations were determined with reference to a standard curve generated with sodium nitrite at various dilutions.
Cytokine Antibody Array
Murine cytokine antibody arrays (M0308003, RayBiotech Inc., Norcross, GA, USA), which detect 62 cytokines on one membrane, were used to determine serum cytokine levels as described previously (35,40). Briefly, the membranes were sequentially incubated with equal volumes of murine serum (after 1:10 dilution), primary biotin-conjugated antibodies, and horseradish peroxidase-conjugated streptavidin. After exposing to X-ray film, the relative signal intensity was determined using the Scion Image software.
Lucifer Yellow Dye Uptake Assay
The Lucifer Yellow dye uptake was used to measure the P2X7R-gated channel activities as described previously (17,45,46). Briefly, RAW 264.7 cells were stimulated with LPS in the absence or presence of CBX or other P2X7R receptor antagonists (KN-62, BBG, or oATP) for 16 h. Subsequently, cell cultures were incubated with Lucifer Yellow (LY, 1 mg/mL) for 15 min, and fixed with 2% paraformaldehyde following three extensive washes with 1 × PBS. The number of cells with diffused fluorescent signals was counted under a fluorescence microscope. The cells containing punctuate fluorescent signals were excluded, as the punctuate signals likely resulted from phagocytosis (rather than passive diffusion through panx-1 hemichannels) of the LY dye.
Animal Model of Polymicrobial Sepsis
This study was approved and performed in accordance with the guidelines of the Institutional Animal Care and Use Committee of the Feinstein Institute for Medical Research, Manhasset, New York, USA. To evaluate the therapeutic potential of CBX, a clinically relevant animal model of sepsis induced by cecal ligation and puncture (CLP) was employed (37,38,47). Briefly, the cecum of BALB/c mice was ligated at 5.0 mm from the cecal tip, and then punctured once with a 22-gauge needle. CBX was administered intraperitoneally into mice at indicated doses and time points, and animal survival rates were monitored for up to 2 wks. In parallel experiments, mice were euthanized to collect blood or peritoneal lavage fluid at 50 h (2 h after the second dose of CBX) after CLP, and assayed for serum levels of TNF, HMGB1 and other cytokines, as described previously (48).
Data are expressed as mean (SEM of two independent experiments in triplicates (n = 2). One-way analyses of variance (ANOVA) followed by the Tukey test for multiple comparisons were used to compare between different groups. The Kaplan-Meier method was used to compare the differences in mortality rates between groups. A P value <0.05 was considered statistically significant.
CBX Dose Dependently Attenuated Endotoxin-Induced HMGB1 Release
The CBX-mediated inhibition of HMGB1 release was not dependent on its cytotoxic activities, as CBX did not reduce cell viability at concentrations up to 20 µmol/L (data not shown). At higher concentrations (50 µmol/L), however, CBX did exhibit noticeable cytotoxicity to RAW 264.7 cells, but not to primary peritoneal macrophages. These observations were consistent with previous findings that prolonged incubation with CBX resulted in cytotoxicity in other tumor cell lines (50). Accordingly, we chose to use nontoxic doses of CBX (10 µmol/L) for most experiments in the present studies unless otherwise noted.
CBX Rescued Mice from Lethal Polymicrobial Sepsis
CBX Selectively Attenuated Sepsis-Induced Local and Systemic HMGB1 Accumulation
CBX Effectively Inhibited P2X7R-Gated Channel Activities
To test this possibility, we determined whether specific P2X7R antagonists similarly inhibit LPS-induced HMGB1 release. As predicted, two selective P2X7R antagonists, oATP and BBG, significantly inhibited LPS-induced LY-uptake in macrophage cultures (Figure 5B). Consistently, both P2X7R antagonists effectively inhibited LPS-induced HMGB1 release (Figure 5C). Surprisingly, another selective P2X7R antagonist, KN62, was ineffective in suppressing LPS-induced LY uptake (see Figure 5B), and similarly failed to inhibit LPS-induced HMGB1 release (see Figure 5C). Taken together, these observations demonstrate a strong correlation between P2X7R-gated channel activity and HMGB1 release in macrophages.
CBX Prevented LPS-Induced PKR Upregulation and Phosphorylation
Many medicinal herbs have been developed into effective therapies for various inflammatory ailments. In this study, we demonstrated that CBX, a derivative of gancao component GZA, effectively inhibited endotoxin-induced HMGB1 release, likely through blocking P2X7R-gated panx-1 channels, and rescued mice from lethal sepsis even when given at relative lower doses (1.2–6 mg/kg) in a delayed regimen (24 h after CLP), possibly through reducing both local and systemic HMGB1 levels.
Since its inception, CBX has been shown to dose dependently inhibit a variety of biological activities including the gap junctions (50–100 µmol/L), panx-1 channels (EC50 = 1–4 µmol/L) (51,52), and 11β-hydroxysteroid dehydrogenase (1–10 µmol/L, 11β-HSD) (53). However, it is unlikely that CBX inhibits LPS-induced HMGB1 release through impairing the gap junctions. First, macrophages did not form gap junctions even after prolonged LPS stimulation, although the cellular panx-1 levels might be elevated (data not shown). Second, the concentrations of CBX used to block gap junctions (for example, 50–100 µmol/L) are much higher than those (for example, 5–10 µmol/L) used to abrogate LPS-induced HMGB1 release. In fact, at relative high concentrations (50–100 µmol/L), CBX exhibited cytotoxicity to RAW 264.7 cells, thereby enhancing (rather than reducing) passive HMGB1 leakage. Thus, it appears that CBX inhibits HMGB1 release through gap junction-independent mechanisms. Similarly, it is unlikely that CBX exerts its inhibition on LPS-induced HMGB1 release through inhibiting 11β-HSD, an enzyme involved in the production of antiinflammatory glucocorticoids. Our previous study indicated that glucocorticoids such as cortisone and dexamethasone were ineffective in inhibiting LPS-induced HMGB1 release in macrophage cultures (40), arguing against the possibility that CBX abrogated HMGB1 release by inhibiting 11β-HSD1.
The possibility for the involvement of panx-1 in CBX-mediated inhibition of HMGB1 release is supported by several lines of evidence. First, unlike other pannexin family members, panx-1 is expressed abundantly on macrophage cytoplasmic membranes. Even though panx-1 may not form gap junctions, it can integrate into hemichannels in macrophages or astrocytes. These panx-1 hemichannels are gated by ATP receptors (for example, P2X7R) and responsible for the increased dye-uptake upon ATP stimulation. Second, as an effective panx-1 channel inhibitor (IC50 < 5 µmol/L), CBX simultaneously inhibited LPS-induced P2X7R/panx-1 channel activation and HMGB1 release, suggesting that the CBX-mediated inhibition of HMGB1 release is likely associated with the blockade of P2X7R-gated panx-1 channel activities. Consistent with this notion, CBX and other panx-1 channel blockers have recently been shown to block HMGB1 release by neurons during cortical spreading depression (54).
Previously, we, and others, have demonstrated that extracellular accumulation of HMGB1 can be attenuated by HMGB1 inhibitors through distinct mechanisms. For instance, mung bean extracts and green tea components (for example, EGCG) prevent extracellular HMGB1 release through stimulating HMGB1 aggregation and autophagic degradation (38,43). Danshen components (for example, tanshinone IIA sodium sulphonate) effectively stimulate endocytic HMGB1 uptake, thereby recycling extracellular HMGB1 back to cytoplasmic vesicles for eventual degradation (36). In a sharp contrast, CBX could neither induce autophagic HMGB1 degradation, nor stimulate endocytic HMGB1 uptake in macrophage cultures (data not shown). Instead, it blocks the LPS-induced activation of P2X7R/panx-1 channels, indicating the selective targeting of LPS-triggered inflammatory signaling cascade in macrophages (see Figure 7). This is noteworthy especially in light of observations that CBX appears to be more effective in blocking the release of HMGB1 than NO and TNF in vitro and in selectively attenuating circulating HMGB1 in septic mice. It is plausible that, as a molecular target of CBX, the P2X7R-gated channels occupy a more important role in the regulation of late (rather than early) mediator of lethal sepsis.
In summary, we have validated the therapeutic potential of CBX in an animal model of polymicrobial sepsis by administering it in a delayed regimen. Furthermore, we have uncovered a novel mechanism by which CBX effectively inhibits HMGB1 release possibly by blocking P2X7R-gated channels and preventing endotoxin-induced PKR activation. Given the central role of PKR in the regulation of inflammasome activation and HMGB1 release, it is important to further delineate the role of P2X7R-gated channels in inflammatory diseases and explore novel PKR-targeting therapeutic strategies.
The authors declare that they have no competing interests as defined by Molecular Medicine, or other interests that might be perceived to influence the results and discussion reported in this paper.
We thank Mala Ashok for assistance with animal experiments, Arvin Jundoria for critical reading of the manuscript, and Kevin J Tracey and Ben Lu for helpful discussions. This work was supported by the National Center of Complementary and Alternative Medicine (NCCAM, R01AT05076) and the National Institute of General Medical Sciences (NIGMS, R01GM063075).
- 47.Li W, et al. (2012) Use of animal model of sepsis to evaluate novel herbal therapies. J. Vis. Exp. (62):3926.Google Scholar
Open Access This article is licensed under a Creative Commons Attribution-NonCommercial-NoDerivatives 4.0 International License, which permits any non-commercial use, sharing, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, and provide a link to the Creative Commons license. You do not have permission under this license to share adapted material derived from this article or parts of it.
The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder.
To view a copy of this license, visit (https://doi.org/creativecommons.org/licenses/by-nc-nd/4.0/)