Acute lung injury (ALI) and its most severe form, acute respiratory distress syndrome (ARDS), is characterized by profound inflammation and tissue injury, often resulting from systemic infections, lung infections, or trauma (1,2). The mortality rate of ALI/ARDS remains unacceptably high, with the average reported in-hospital mortality rate ranging from 30% to 50%. In addition to increased mortality during and after hospital discharge, patients who survive ARDS are likely to experience significant long-term sequelae (3).
Macrophages are key contributors to both the induction and resolution of lung inflammation (4). Based on their phenotype and function, macrophages have been broadly classified into classically activated (M1) and alternatively activated (M2) macrophages. Macrophages are polarized to the M1 phenotype by interferon-γ or lipopolysaccharide (LPS) and this phenotype is generally characterized by a high production of pro-inflammatory factors, such as interleukin 1β (IL-1β), IL-6, IL-12, tumor necrosis factor-α (TNF-α), and inducible nitric oxide synthase (iNOS). M1 macrophages are important for the direct host-defense against pathogens (5,6). The M2 phenotype is induced by exposure to IL-4, IL-13, IL-10, as well as glucocorticoids, and its hallmark is the production of anti-inflammatory molecules, including IL-10, found in the inflammatory zone (Fizz-1), chitinase-like 3 (Ym-1), and arginase-1 (Arg-1). In contrast to M1 macrophages, M2 macrophages coordinate a series of regulated responses to abrogate inflammation and enhance tissue repair (5-8).
A growing number of studies have shown that macrophage M1/M2 imbalance is implicated in the development and recovery of ALI. For example, neutrophil extracellular traps (NETs) promote ARDS inflammation during the acute phase by inducing macrophage polarization to the M1 phenotype (9). MCP-induced protein 1 (MCPIP1) plays a protective role in sepsis-induced ALI by modulating macrophage polarization to the M2 phenotype via inhibition of the JNK/c-Myc signaling pathway (10). Moreover, the promotion of the M2 phenotype was shown to have a protective role in endotoxemia and LPS-induced ALI (11,12). These findings suggest that inhibition of M1 and/or promotion of M2 may have a critical therapeutic value in alleviating ALI.
Endoplasmic reticulum (ER) stress is defined as the accumulation of unfolded or misfolded proteins in the ER, which induces a coordinated adaptive process called the unfolded protein response (UPR). In mammalian cells, the UPR pathway involves three primary signaling cascades initiated by the ER-localized transmembrane proteins: the protein kinase receptor-like ER kinase (PERK), proto-transcription factor activating transcription factor 6 (ATF6), and inositol-requiring enzyme-1 (IRE-1). In response to ER stress, PERK activation regulates cellular protein synthesis via phosphorylation of the eukaryotic translation initiation factor 2α (eIF2α). IRE-1 triggers changes in downstream signaling by splicing 26 nucleotides from the XBP-1 mRNA, thereby causing a frameshift in its translation. ATF-6 leaves the ER and traffics to the Golgi, where it is processed to an active form. Activation of these signaling cascades leads to the upregulation of various UPR target genes to restore ER homeostasis (13).
In addition to its intrinsic effects on protein translation and folding, ER stress is linked to lung inflammatory diseases. A number of studies have shown that GRP78, an ER stress marker and UPR mediators are enhanced in both ALI/ARDS patients and rodent models of LPS-induced ALI (14-16). Moreover, inhibition of ER stress has been shown to alleviate endotoxin-induced ALI both in vivo and in vitro, thereby underlining the potential importance of this pathway in lung inflammation (15,16). Thus, ER stress may be a central component of lung inflammatory diseases.
Therefore, both ER stress and M1/M2 imbalance contribute to inflammatory processes in lung injury. However, little is known regarding the interaction between ER stress and M1/M2 imbalance in lung inflammation. In this study, we evaluated the possible role of the M1/M2 imbalance in LPS-induced lung inflammation, focusing on the crosstalk between ER stress and macrophage phenotype change in LPS-induced ALI.
LPS (Escherichia coli 055:B5), tauroursodeoxycholic acid (TUDCA), and 4µ8c were purchased from Sigma (St. Louis, MO, USA). Recombinant M-CSF and IL-4 were purchased from PeproTech (Rocky Hill, NJ, USA). All cell culture reagents were purchased from Invitrogen (Carlsbad, CA, USA). The protease and phosphatase inhibitor cocktails, BCA protein assay kit, enhanced ECL chemiluminescence reagent, and Western blot stripping buffer were purchased from Thermo Scientific (Rockford, IL, USA). Anti-GRP78 and anti-ATF6 antibodies were purchased from Abcam (Cambridge, MA, USA), while anti-XBP-1s, anti-eIF2α, and anti-p-eIF2α antibodies were purchased from Cell Signaling Technology (Danvers, MA, USA). The β-actin-peroxidase mAb was purchased from Sigma-Aldrich. PE-labeled Arg-1 was purchased from R&D Systems (Minneapolis, MN, USA), and eFluor 660-labeled CD170 (Siglec F), FITC-labeled CD11c, and PE-Cy7 labeled iNOS were purchased from Affymetrix eBioscience (San Diego, CA, USA).
Male C57BL/6 mice (8–10-week-old) were purchased from Bi Kai Experimental Animals (Shanghai, China) and bred in the Animal Care Facility of Tongji University affiliated with the Shanghai Pulmonary Hospital. LPS-induced ALI was performed as previously described (11). Briefly, following anesthetization with pentobarbital, 50 µg of LPS in a volume of 25 µL of saline was delivered to the mice intratracheally using a MicroSprayer syringe assembly (MSA-250-M, Penn Century, USA). ALI control mice (Veh) received the same amount of sterile saline. For TUDCA treatment, a dose of 5 mg/kg of TUDCA was administered intraperitoneally 1 h before LPS treatment. Vehicle control mice received the same amount of sterile saline. At specific time points following LPS administration, the bronchoalveolar lavage fluid (BALF) and lung tissue samples were obtained for Western blotting and quantitative RT-PCR analysis. In separate experiments, nonlavaged lungs were collected for histological study.
Immediately after being sacrificed by administering an anesthetic overdose, 500 µL of PBS were slowly infused in the murine lungs via tracheostomy and, then, withdrawn gently. This lavage was repeated 3 times and the obtained BALF samples were mixed. The fluid was, then, centrifuged and the cell-free supernatant was aliquoted and stored at −80 °C until use. For the pellet, total cells were either counted on a hemocytometer following lysis of erythrocytes or purified by adhesion to tissue culture plastic to obtain alveolar macrophages (AMs) (17).
Bone marrow-derived macrophage (BMDM) culture
Bone marrow cells were collected from the femurs and tibias of C57BL/6 mice and treated with a red blood cell lysis buffer. The remaining cells were cultured in DMEM medium supplemented with 10% (vol/vol) fetal bovine serum, M-CSF (20 ng/mL), penicillin (100 U/mL), and streptomycin (100 U/mL). On day 6 or 7, BMDMs were replated and then untreated (M0) macrophages were stimulated with LPS (100 ng/mL) for 18 h (M1), or with IL-4 (20 ng/mL) for 18 h (M2). To induce ER stress, BMDMs were pretreated with 2.5 µM thapsigargin (Tg) for 1 h. To inhibit ER stress and XBP-1 splicing, BMDMs were pretreated either with 50 µg/mL TUDCA or 5 µM 4µ8c (18) for 1 h. After stimulation, cells were harvested and stained for flow cytometry analysis or subjected to quantitative RT-PCR analysis.
Western blot analysis
Cell and lung samples were homogenized in RIPA buffer containing protease and phosphatase inhibitor cocktails. The total protein content in the tissue lysates was quantified using the BCA protein assay kit. Equal amounts of protein samples were separated by SDS-PAGE. Proteins were, then, transferred to a PVDF membrane (Bio-Rad, Hercules, CA, USA). The membranes were incubated overnight at 4 °C with primary antibodies diluted in TBST (TBS containing 0.1% Tween-20) buffer containing 3% non-fat milk, followed by incubation with corresponding secondary antibodies for 1 h at room temperature. Immunoreactive bands were detected using the enhanced ECL chemiluminescence reagent. The membrane was stripped using the Western blot stripping buffer and subsequently labeled with β-actin antibodies following the procedure described above. Immunoreactive bands were captured using the Amersham Imager 600 software (GE Healthcare).
RNA isolation and quantitative RT-PCR
Total RNA was isolated using the TRIzol reagent (Invitrogen, Carlsbad, CA, USA), following the manufacturer’s instructions. Along with genomic DNA (gDNA) removal, 500 ng of RNA was reverse transcribed using the TransScript All-in-One First-Strand cDNA Synthesis Kit (Transgenbiotech, Beijing, China). RT-PCR (SYBR) was performed using reagents from Transgenbiotech (Beijing, China) on a QS6 Real-Time PCR System (Applied Biosystems). Relative gene expression levels were calculated using the comparative threshold cycle (Ct) method and normalized to β-actin. The primers used for amplification are listed in Table 1.
Determination of cytokine levels
IL-1β, IL-6, IL-10, IL-12, MIP-1α, and TNF-α levels in the BALF samples were measured by Luminex 200 (Bio-Rad, Hercules, CA, USA).
Lung histological study
Following treatment with TUDCA and LPS, mice were sacrificed by administering an anesthetic overdose. The left lungs were harvested and fixed with 4% paraformaldehyde. After tissue embedding and sectioning, lung slices were subsequently stained with hematoxylin and eosin (H&E). The tissue sections were observed under a light microscope and images were captured using an Olympus IX73 microscope (Clarksburg, NJ, USA). To perform the histological assessment of lung injury, five independent variables were evaluated—interstitial edema, hemorrhage, neutrophil infiltration, atelectasis, and necrosis. The severity of injury was judged by an investigator blinded to the experimental protocol according to the following criteria: no injury =0; injury to 25% of the field =1; injury to 50% of the field =2; injury to 75% of the field =3 and diffuse injury =4 (19,20).
Flow cytometry analysis
Cells isolated from BALF samples were first incubated with Fc block (eBioscience) and, then, cell surface staining was carried out by incubation with APC-conjugated anti-mouse CD11c and FITC-conjugated anti-mouse Siglec F. Following fixation and permeabilization (BD Fixation and Permeabilization Solution Kit, BD Biosciences), intracellular staining was performed by incubation with PE-conjugated anti-mouse Arg-1 and PE-CY7-conjugated anti-mouse iNOS. The proper isotype controls were used in each case. Flow cytometry events were gated first based on forward and side scatter. Then, CD11c+ Siglec F+ cells (21,22) (for in vivo AMs) were selected to evaluate the expression of Arg-1 and iNOS, respectively. Each flow cytometry analysis experiment was run on at least 100,000 cells and data were acquired using a BD FACSCantoTM II instrument and analyzed using the FlowJo X software.
All data, unless otherwise indicated, are presented as the mean ± standard deviation (SD) of independent experiments. The statistical significance of the differences between the two groups was analyzed using Student’s t-test. A P value of ≤0.05 was considered to be statistically significant. All statistical analyses were performed using the GraphPad Prism 8 software program for Windows.
ER stress and the UPR signaling pathway were activated in LPS-induced ALI
To investigate whether ER stress is involved in LPS-induced lung injury, we measured the protein levels of GRP78 and various UPR markers in a murine model of LPS-induced ALI. Within hours of tracheal instillation of LPS, mice developed severe lung injury characterized by increased protein concentrations and number of inflammatory cells in BALF samples when compared with those of vehicle mice (Figure 1A,B,C). Macrophage and neutrophil infiltration increased within 6 h after LPS administration and reached peak levels at 24 h. A full recovery was achieved at day 11 (Figure 1B,C). Protein concentrations in the BALF also peaked at 24 h and significantly decreased on day 7 and 11 (Figure 1A). Consistently, histological analysis showed that the severity of lung injury, characterized by thickening of the alveolar septum, inflammatory cell infiltration, and alveolar fusion, peaked at 24 h after LPS administration and declined thereafter (Figure 1D,E).
We subsequently analyzed changes in ER stress mediators during the induction and resolution phases of ALI. As shown in Figure 1F, the protein expression of GRP78 was increased by LPS administration at 6 h, peaked at 24 h and returned to the normal level on day 7 and 11. To further investigate which UPR components are involved in LPS-induced ER stress, three key proteins, ATF6, XBP-1, and phosphorylated eIF2α (p-eIF2α), were detected by Western blotting. We found that the expression of p-eIF2α and ATF6 proteins did not change significantly after LPS treatment, whereas LPS treatment induced the accumulation of spliced XBP-1 (XBP-1s) in lung tissues. This suggests that ER stress and IRE-1/XBP-1 signaling play an important role in LPS-induced ALI.
Macrophage diversity was detected in the induction and resolution phase of ALI
Considering that macrophage polarization is closely associated with lung inflammation and that M1-polarized macrophages exhibit a pro-inflammatory phenotype, we identified the phenotype of infiltrated macrophages in the LPS-induced ALI model. The concentration of inflammatory mediators in the BALF peaked at either 6 or 24 h following LPS administration and returned to basal levels on day 11 (Figure 2A). We also examined the gene expression levels of M1 and M2 markers in RNA isolated from AMs. As expected, the gene expression level of M1 markers (IL-1β, IL-6, IL-12, and TNF-α) peaked early at 6 h during the acute phase of inflammation and injury (Figure 2B). Unlike the M1 markers, the trends seen in the expression of M2 markers were different. Fizz-1 appeared to have a bimodal distribution (Figure 2B) and peaked during both the induction and resolution phases of lung inflammation. Arg-1 expression peaked on day 3, while Ym-1 mRNA was significantly suppressed at 6 and 24 h after LPS administration and gradually returned to basal levels on day 11. Our results indicate that the AM population polarizes to an inflammatory M1 phenotype in the acute phase of inflammation and gradually shifts to an M2 phenotype in the resolution phase. Further, these results suggest that M1/M2 imbalance plays an important role in the development and resolution of ALI.
ER stress inhibitor TUDCA attenuated LPS-induced ALI by mitigating M1 macrophage polarization
We next investigated the inhibitory effects of TUDCA (23), a potent ER stress inhibitor, on LPS-induced lung inflammation. As shown in Figure 3A, TUDCA treatment inhibited the protein expression of GRP78 and XBP-1s in LPS-instilled mice. Histological analysis revealed that LPS caused a significant increase in the inflammatory infiltrating cells and structural damage when compared with the vehicle control. However, TUDCA treatment attenuated these histological changes (Figure 3B). We also found that TUDCA treatment prevented lung vascular permeability in ALI, as assessed by the protein concentration in BALF samples (Figure 3C). The same trends were observed for the number of inflammatory cells in BAFL samples (Figure 3D) and inflammatory mediator levels in lung tissues (Figure 3E). At 24 h following LPS administration, the total number of cells in BALF samples and mRNA levels of IL-1β, IL-6, IL-10, and TNF-α were significantly increased. Following TUDCA administration, IL-10 levels slightly increased, while the total number of cells and IL-1β, IL-6, and TNF-α levels decreased remarkably, indicating attenuated inflammation (Figure 3D,E). Consistent with these observations, flow cytometry analysis revealed a decreased expression of the M1 activation marker iNOS in the TUDCA treatment group when compared to the LPS group (Figure 3F). Moreover, TUDCA treatment did not promote the expression of the M2 activation marker Arg-1. There was no statistical difference between the vehicle and TUDCA administration alone groups.
ER stress promoted M1 polarization and the switch from the M2 phenotype to the M1 phenotype in BMDMs
To investigate how ER stress affects macrophage polarization, we treated BMDMs with the ER stress-inducing drug, Tg, followed by polarization to the M1 and M2 phenotypes. We found that induction of ER stress caused a further increase in the expression of pro-inflammatory M1 markers (IL-1β, IL-6, and TNF-α) in response to LPS stimulation. However, the gene expression of M2 markers (Fizz-1, and Ym-1) was inhibited in the presence of Tg (Figure 4A). Similarly, flow cytometry analysis revealed that Tg significantly enhanced iNOS expression in LPS-stimulated BMDMs, as shown by the right shift of the curve in the presence of Tg, but inhibited Arg-1 expression in IL-4-stimulated BMDMs (Figure 4B).
Blockade of ER stress and the XBP-1 signaling pathway inhibited M1 polarization in BMDMs
To further confirm that ER stress promotes M1 polarization, we investigated the effects of an ER stress inhibitor on macrophage phenotype. Furthermore, we also evaluated whether the XBP-1 signaling pathway is involved in the macrophage phenotype shift. As expected, treatment with TUDCA and 4µ8c, which block substrate access to the active site of IRE-1α and selectively inactivates XBP-1 splicing (18), respectively, inhibited LPS-induced M1 marker expression (IL-1β, IL-6, and TNF-α) (Figure 5A), but did not further enhance IL-4-induced M2 marker gene expression (Fizz-1, and Ym-1) in BMDMs (data not shown here). Consistent with these observations, flow cytometry analysis showed that treatment with both TUDCA and 4µ8c significantly decreased the gene expression of iNOS in LPS-stimulated BMDMs, but did not enhance the gene expression of Arg-1 in IL-4-stimulated BMDMs (Figure 5B). There was no statistically significant difference between the M0, TUDCA, and 4µ8c treatment alone groups (Figure 5A).
ALI/ARDS, caused by either direct or indirect lung insults, can result in uncontrolled lung inflammation and structural changes that are associated with high morbidity and mortality (1,2). Macrophage diversity contributes to both the promotion and resolution of lung inflammation. ER stress is a potent evolutionarily conserved response to misfolded proteins resulting from cellular stresses, such as inflammation. In this study, we demonstrated for the first time that the ER stress-mediated M1/M2 imbalance plays a role in promoting inflammation in ALI. Furthermore, we showed that inhibition of the ER stress-associated IRE-1/XBP-1 pathway suppresses M1 polarization, thus alleviating ALI.
ER stress has been implicated in a variety of diseases, including diabetes, atherosclerosis, neurodegenerative diseases, cancer, and inflammatory diseases (24,25). In particular, several studies have suggested a potential role of ER stress in the pathogenesis of lung injury. Saurabh and colleagues showed that patients with severe chronic obstructive pulmonary disease have elevated levels of the ER stress marker GRP78 (26). Enhancement of ER stress has been associated with the pathogenesis of idiopathic pulmonary fibrosis (27). In addition, ER stress is involved in LPS-induced lung injuries in vivo and is enhanced in LPS-stimulated airway epithelial cells and thrombin-stimulated endothelial cells in vitro (15,16,28). Our results also showed that the GRP78 protein levels were significantly increased following LPS administration at 6 h and peaked at 24 h. Among the three UPR mediators, p-eIF2alpha, XBP-1, and ATF-6, only XBP-1s was significantly elevated in the lung tissues of LPS-treated mice. Furthermore, increased inflammatory cell infiltration and proinflammatory mediator secretion, as well as structural damage were observed in the lung of LPS-instilled mice. Moreover, we found that TUDCA, a potent ER stress inhibitor, markedly reduced the LPS-induced upregulation of GRP78 and XBP-1s in mice, as well as inhibited lung inflammation and histological changes. These findings suggest that the ER stress-associated XBP-1 pathway is one of the crucial players in the induction and maintenance of LPS-induced lung inflammation and that TUDCA attenuates ER stress in ALI.
Accumulating evidence has suggested that macrophage diversity is a key regulator of the development and recovery of ALI/ARDS and that different macrophage subtypes play different roles at different stages of ALI/ARDS (4,22,29). Therefore, we analyzed the macrophage phenotype in a mouse model of LPS-induced lung injury. We found that the production of pro-inflammatory mediators (IL-1β, IL-6, IL-12, MIP-1α, and TNF-α) in BALF samples peaked at either 6 or 24 h following LPS administration. Interestingly, IL-10 levels were also elevated, possibly as a result of a large release of pro-inflammatory factors that activate anti-inflammatory responses. Moreover, the mRNA of pro-inflammatory M1 markers (IL-1β, IL-6, IL-12, and TNF-α) peaked at 6 h, during the acute phase of inflammation and injury. Unlike the M1 markers, the M2 gene panels (Fizz-1, Arg-1 and Ym-1) showed a different expression trend and were mostly enhanced in the resolution phase. Our data suggest that the AM population polarizes to an inflammatory macrophage phenotype upon exposure to LPS in the induction phase and to an anti-inflammatory macrophage phenotype in the resolution phase. Thus, restoring the M1/M2 imbalance via inhibition of the M1 phenotype and/or promotion of the M2 phenotype may have a critical therapeutic value in alleviating ALI.
Both ER stress and M1/M2 imbalance are potential therapeutic targets for various inflammatory diseases. Based on our current results, we speculate that ER stress may play a role in promoting M1 macrophage polarization. As expected, we found that Tg treatment caused either a further increase in pro-inflammatory M1 marker gene expression or a further decrease in anti-inflammatory M2 marker gene expression in BMDMs. In contrast, blockade of ER stress via TUDCA treatment generated the opposite effect in M1 signature markers but did not promote M2 signature markers. Consistent with the effect of TUDCA on macrophage polarization, the IRE-1 endonuclease inhibitor also demonstrated an inhibitory effect on M1 markers but did not promote the expression of M2 markers. These observations indicate that the blockade of the ER stress-associated IRE-1/XBP-1 signaling pathway alleviates ALI by inhibiting M1 polarization.
There are several limitations to our study. First, we could not address the cause-effect relationship between ER stress and inflammatory mediator secretion. Several studies indicate that not only does ER stress amplify inflammatory reactions but also that pro-inflammatory mediators, such as IL-1β, IL-6, TNF-α, and IL-17, contribute to the induction of ER stress (15,30-32). Our study demonstrated that inhibition of ER stress suppresses LPS-induced inflammation. Second, a proof-of-concept study is needed to determine the causal role of XBP-1 signaling in LPS-induced ALI using XBP-1 transgenic mice.
Taken together, our results demonstrate that inhibition of the ER stress-associated IRE-1/XBP-1 signaling pathway suppresses macrophage polarization to the M1 phenotype and ameliorates LPS-induced lung inflammation and injury. Moreover, our results suggest that the interaction between ER stress and macrophage phenotype might be a novel therapeutic target for endotoxin-induced lung inflammatory disorders.
Funding: This work was supported by the National Natural Science Foundation of China (No. 81400056 to Y Zhao, 81100061 to W He, 81670089 to W He and 81900078 to L Chen), Shanghai Municipal Commission of Health and Family Planning (No. 201540161 to Y Zhao, and 201640225 to W He).
Conflicts of Interest: The authors have no conflicts of interest to declare.
Ethical statement: The authors are accountable for all aspects of the work in ensuring that questions related to the accuracy or integrity of any part of the work are appropriately investigated and resolved. All animal protocols were approved by the Animal Care and Use Committee of Shanghai Pulmonary Hospital (No. 2014fk12) and met the standards of the Institutional Health Guide for care and use of laboratory animals.
Open Access Statement: This is an Open Access article distributed in accordance with the Creative Commons Attribution-NonCommercial-NoDerivs 4.0 International License (CC BY-NC-ND 4.0), which permits the non-commercial replication and distribution of the article with the strict proviso that no changes or edits are made and the original work is properly cited (including links to both the formal publication through the relevant DOI and the license). See: https://creativecommons.org/licenses/by-nc-nd/4.0/.
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