Linarin prevents LPS-induced acute lung injury by suppressing oxidative stress and inflammation via inhibition of TXNIP/NLRP3 and NF-κB pathways

Abstract

Acute lung injury (ALI) is an important cause of morbidity and mortality for critically ill patients, and linarin (LR) may be a potential treatment for ALI as it reportedly has antioxidant, anti-inflammatory and apoptotic-regulating activity. In the present study, the authors report that saline and LR (12.5, 25 and 50 mg/kg) were applied to male C57BL/6 mice via gavage. Then, mice were intratracheally injected with either saline or lipopolysaccharide (LPS). LR-pretreatment attenuated LPS-induced ALI and platelet activation and reduced CD41 expression levels and neutrophil platelet aggregates. Additionally, LPS-triggered pulmonary myeloperoxidase activity and neutrophil infiltration in lung tissues, and this was eliminated by LR dose-dependently. Furthermore, LPS-induced oxidative stress and pro-inflammatory cytokine release were downregulated by LR by inhibiting thioredoxin-interacting protein and nuclear factor-κB signaling pathways, including their downstream and upstream signals, such as xanthine oxidase, NLR family WHAT, pyrin domain-containing 3 (NLRP3), apoptosis-associated speck-like protein containing a C-terminal caspase recruitment domain (ASC), caspase-1, IκB kinase-α (IKK-α) and IκBα. Moreover, in LPS-induced mice, the mitogen-activated protein kinase pathway was inactivated by LR. In vitro, LR reduced LPS-induced inflammation and oxidative stress, which was linked to reduction of ROS. In conclusion, LR pretreatment may be protective against LPS-induced ALI.

Introduction

Acute lung injury (ALI) and acute respiratory distress syndrome (ARDS) are life-threatening diseases induced by severe sepsis, severe bacterial pneumonia, trauma and burns (1,2). Although advances have been made in understanding the pathophysiology of ALI and ARDS, there is no effective therapeutic strategy for treating either (3). Various molecular mechanisms are associated with the pathogenesis and progression of ALI, including oxidative stress and inflammatory responses (4). ALI is characterized by extreme inflammation, excessive neutrophil infiltration into the lung tissues, release of pro-inflammatory cytokines, and lung endothelial and epithelial injuries, resulting in edema and gas exchange deterioration (5,6).

Reactive oxygen species (ROS)-induced oxidative stress contributes to ALI development (7) via stimulating TXNIP/NLRP3, nuclear factor (NF)-κB and mitogen-activated protein kinase (MAPK) signaling pathways (8). TXNIP/NLRP3 activation is linked to ALI and TXNIP blocks antioxidant function; its overexpression has been observed in diverse diseases (9,10). Accumulating evidence indicates that the NLRP3 inflammasome initiates the innate immunity and promotes inflammatory responses (11). Importantly, TXNIP links oxidative stress to NLRP3 activation in an ROS-sensitive manner (12). The process accelerates the secretion of pro-inflammatory cytokines, including tumor necrosis factor (TNF)-α, interleukin (IL)-1β and IL-6, which are associated with NF-κB activity, eventually contributing to ALI (13). MAPKs are implicated in cellular inflammatory processes in response to oxidative stress (14).

LR (LR; acacetin-7-O-β-D-rutinoside) is a natural flavonoid glycoside abundant in various vegetables and fruits (15). Plants containing LR have been reportedly used to treat inflammatory diseases, cancer and hypertension (16,17). LR alleviates LPS-induced cytokine production in a murine macrophage cell line (18). Recently, LR was reported to have antioxidant activity associated with enhancement of nuclear factor-erythroid 2-related factor 2 (Nrf2). LR activated Nrf2 activation to reduce ROS generation, inhibiting ischemia-reperfusion injury (19). Thus, LR may have potential for use in the treatment of ALI.

The current study reports that LPS induced ALI, as evidenced by platelet activation, inflammation and oxidative stress via activating NF-κB and TXNIP/NLRP3 pathways, was suppressed by linarin partly via suppressing NF-κB and TXNIP/NLRP3, and by potentiating Nrf2. Therefore, LR pretreatment may prevent ALI-induced by LPS in vitr and in vivo.

Materials and methods

Animals and treatment

A total of 100 male C57BL/6 mice (6–8 weeks old, weighing, 18–20 g) were purchased from The Animal Center of Nanjing Medical University (Nanjing, China), and provided with food and water ad libitu and kept in climate-controlled quarters with a 12 h light/dark cycle with food and water in cages under the germ-free conditions at a temperature of 25°C. The mice were housed for a minimum of one week for environmental adaptation prior to experimentation. All procedures were in accordance with the Regulations of Experimental Animal Administration issued by the Ministry of Science and Technology of the People's Republic of China, and before the animal experiments were performed, the procedures were approved by the Research Ethical Committee of Huai'an First People's Hospital, Nanjing Medical University (Nanjing, China).

C57BL/6 mice were randomly divided into 5 groups as follows (n=20 in each group): i) Control (Con); ii) LPS treatment (LPS); iii) Low dose of LR treatment (LPS treatment + oral gavage of 12.5 mg/kg LR for 3 days, LD-LR); iv) Medium dose of LR treatment (LPS treatment + oral gavage of 25 mg/kg LR for 3 days, MD-LR); and v) High dose of LR treatment (LPS treatment + oral gavage of 50 mg/kg LR for 3 days, HD-LR). The mice from the control and LPS groups received an equal volume of normal saline (0.3 ml) instead of LR. LR was purchased from Fanke Biotech Fanke Biotech Co., Ltd. (http://fanketech.biomart.cn, FA-1701, HPLC ≥98%, Shanghai, China). At 3 h following drug administration on the third day, the mice were slightly anesthetized with inhalation of diethyl ether (1 ml diethyl ether dipping cotton balls), and 10 µg LPS in 50 µl PBS was intranasally instilled to induce lung injury. The mice in the control group were given 50 µl normal saline in the absence of LPS. A total of 24 h later for LPS treatment, all mice were sacrificed through an intraperitoneal injection of 50 mg/kg pentobarbital (Sigma-Aldrich; Merck KGaA, Darmstadt, Germany) and bronchoalveolar lavage fluid (BALF) and lung tissue samples were harvested for further researches. The ratios of lung wet/dry weight were measured by dividing the wet weight by the dry weight. The middle lobe of the right lung was excised and the wet weight was recorded. Then, the lung was placed in an incubator for 24 h at 80°C to obtain the dry weight.

Cells and culture

Thehuman lung epithelial cell line, BEAS-2B, was purchased from Shanghai Haoran Biological Technology Co., Ltd. (Shanghai, China) and kept in DMEM/F12 containing 1% penicillin/streptomycin and 10% FBS (Hyclone; GE Healthcare Life Sciences, Chalfont, UK). Cells were then cultured in a humidified atmosphere with 5% CO₂ and 95% humidity at 37°C in an incubator.

Biochemical assays

Superoxide dismutase (SOD, A001-3), catalase (CAT, A007-1-1) and glutathione peroxidase (GPx, A005) activities, as well as malondialdehyde (MDA, A003-1) levels in lung tissue sample were determined by commercially available kits (Nanjing Jiancheng Bioengineering Institute, Nanjing, China) following the manufacturer's instructions. H₂O₂ levels in lung tissues were measured using a hydrogen peroxide assay kit, (Beyotime Institute of Biotechnology, Haimen, China) following the manufacturer's instructions. O₂⁻ in lung tissues was measured through lucigenin chemiluminescence method. Briefly, lung tissues of mice under different conditions were weighed and homogenized in a homogenization buffer using HEPES and EDTA. Following centrifugation (1,000 × g at 4°C for 10 min), an aliquot of the supernatant was incubated with 5 µM lucigenin in Krebs-HEPES buffer. Light emission was measured with a Tecan Infinite 200 (Tecan Group AG, Männedorf, Switzerland). Specificity for O₂⁻ was evaluated by adding SOD (350 U/ml) to the incubation medium. BCA Protein Quantitative Analysis kit (Thermo Fisher Scientific, Inc., Waltham, MA, USA) was used to measure the protein concentration.

Assessment of arterial blood gas

A total of 40 male C57BL/6 mice (6–8-weeks old, 18–20 g weight) were pretreated with LR (0, 12.5, 25 and 50 mg/kg) for 3 days by gavage orally. At 3 h following drug administration on the third day, the mice were slightly anesthetized with inhalation of diethyl ether (1 ml diethyl ether dipping cotton balls), and 10 µg LPS in 50 µl PBS was instilled intranasally to induce lung injury. The mice in the control group were given 50 µl of normal saline without LPS. At 24 h following LPS treatment, the mice were sacrificed by an intraperitoneal injection of pentobarbital (50 mg/kg; Sigma-Aldrich; Merck KGaA). The retro-orbital blood samples (1 ml) from each mouse was collected and used to measure the parameters of arterial blood gas, including blood hemoglobin concentration (Hgb), pH, HCO₃, partial pressure of oxygen (PO₂), partial pressure of carbon dioxide (PCO₂), lactate (LAC) and base excess (BE) using Hitachi 8500 automatic analyzer (Hitachi, Ltd., Tokyo, Japan).

Immunofluorescence analysis

For measurement of CD41 using immunofluorescence staining was performed. Briefly, the frozen sections of lung tissue samples were washed with PBS twice and then were blocked with 1% bovine serum albumin at room temperature for 30 min. Then the cells and heart tissue samples were incubated overnight with rabbit anti-CD41 primary antibody (ab63983, 1:50; Abcam, Cambridge, UK). After being washed with PBS for three times, the samples were performed with goat anti-rabbit secondary antibody conjugated to Alexa Fluor 647 (A0468, 1:400) and goat anti-rabbit secondary antibody conjugated to Alexa Fluor 488 (A0423, 1:400) (both from Beyotime Institute of Biotechnology) for 1 h under dark conditions. Then, the cells were counterstained with DAPI (Beyotime Institute of Biotechnology) for 15 min, and the tissue sections were analyzed using an immunofluorescence microscope. Three slides per experimental condition are repeated three times.

Bronchoalveolar lavage fluid (BALF) isolation and analysis

BALF was collected by flushing the left lung (0.4 ml, three times). Total BALF cells were measured using a hemocytometer. A part of the BALF was centrifuged for 5 min at 92 × g by cytospin on a microscopic slide at 4°C. BALF cells were stained using Giemsa at room temperature for 10 min. The rest of BALF was filtrated through a 0.22 µm pore-size filter and then stored at −80°C for protein and cytokine detection, while the cell pellet was resuspended in PBS for counting the neutrophils. The concentration of BALF protein was measured using BCA Protein Assay kit.

Measurement of cytokine levels in BALF

IL-1β (cat. no. MLB00C), TNF-α (cat. no. MTA00B), IL-10 (cat. no. DY417), IL-6 (cat. no. M6000B), cyclooxygenase (COX)2 (cat. no. DYC4198-2), monocyte chemotactic protein 5 (MCP-5; cat. no. MCC120), macrophage inflammatory protein-1α (MIP-1α) (cat. no. MMA00), thromboxane B2 (TXB2; cat. no. KGE011) and myeloperoxidase (MPO; cat. no. DY3667) levels in BALF were measured using ELISA kits (R&D System Inc., Minneapolis, MN, USA). The procedures were performed following the manufacturer's instructions.

Immunohistochemical analysis

Histopathological evaluation was performed on mice not subjected to BAL. Lungs were inflated and fixed with 10% buffered formalin for 48 h at room temperature and embedded in paraffin (Beyotime Institute of Biotechnology). Tissue sections were cut at 4 µm thickness and stained with hematoxylin and eosin (H&E) following the regular staining method. The sections were deparaffinized in xylene for 10 min. Then, the slides were re-hydrated in absolute alcohol for 5 min each, followed by 95% alcohol for 2 min and 70% alcohol for 2 min and then washing with water. Subsequently, the sections were stained in Harris hematoxylin solution for 8 min at room temperature, followed by washing under a running water for 5 min. The slides were then differentiated in 1% acid alcohol for 30 sec, followed by washing using running tap water for 1 min. Then, the sections were subjected to bluing in 0.2% ammonia water or saturated lithium carbonate solution for 30 sec at room temperature, followed by washing under running water for 5 min and rinsing in 95% alcohol. The sections were counterstained in eosin-phloxine solution for 30 sec at room temperature; the slides were dehydrated via 95% alcohol for 5 min and cleared in xylene for 5 min. Finally, the sections were mounted with xylene-based mounting medium. The severity of injury was judged based on the following criteria: 0, no injury; 1, injury to 25% of the field; 2, injury to 50% of the field; 3, injury to 75% of the field; and 4, diffuse injury. The ultimate score was obtained by adding the aforementioned scores. Immunohistochemistry was performed using the paraffin-embedded tissue sections at 4 µm thickness mounted on glass slides. The slides were then deparaffinized and rehydrated. Then, the lung sections were incubated with primary antibodies against mouse TXNIP (ab210826, dilution: 1:200) and xanthine oxidase (XO, ab176165, dilution: 1:200) (both from Abcam), and then with biotin secondary antibodies (B3640; Sigma-Aldrich; Merck KGaA) at room temperature for 30 min. The number of XO-, and TXNIP-positive cells in lung sections was counted using Pax-it software (version 6; Paxcam, Villa Park, IL, USA).

Flow cytometry assays

Whole blood samples from mice were collected and maintained in acid citrate dextrose (Sigma-Aldrich; Merck KGaA). Anti-CD11b eFluor450 (1:100), anti-CD41-allophycocyanin (1:100) (both from eBioscience; Thermo Fisher Scientific, Inc.), anti-Ly6C-PE (1:100; BD Biosciences, Franklin Lakes, NJ, USA) and anti-Ly6G-phycoerythrin (1:100; BD Biosciences) were used to detect leukocyte and platelets antigens. Samples were examined with an LSRII flow cytometer (BD Biosciences) and analyzed using FCS express software (version 3.0, De Novo Software, Glendale, CA, USA). Neutrophils and monocytes were gated through their forward- and side-scatter characteristics and through their Ly-6G⁺/CD11b⁺ (neutrophil) and Ly-6G⁻/CD11b⁺/Ly-6C⁺ (monocyte) expression pattern. Platelet-neutrophil and platelet-monocyte aggregates were calculated using CD41 antibody staining.

ROS generation

Intracellular ROS generation regulated by LPS, ATP and N-Acetylcysteine (NAC) (both from Sigma-Aldrich; Merck KGaA) was assessed by calculating the fluorescence intensity of 2′,7′-dichlorofluorescein diacetate oxidized product (Molecular Probes; Thermo Fisher Scientific, Inc.). The relative fluorescence intensity of oxidized product of 2′,7′-dichlorofluorescein diacetate, was tested at an excitation wavelength of 485 nm and an emission wavelength of 530 nm using a Quantus™ Fluorometer (Promega Corporation, Madison, WI, USA). All cells after various treatments were harvested for ROS assessment through ROS Fluorescent Probe-DCF (Vigorous Biotechnology Beijing Co., Ltd., Beijing, China;http://www.vigorousbiol.com/) according to the manufacturer's instructions.

Reverse transcription-quantitative (RT-qPCR) analysis

Lung samples were immediately acquired from mice following sacrifice and were used in the extraction of total RNA using TRIzol reagent (Invitrogen; Thermo Fisher Scientific, Inc.). Subsequently, the RNA was purified using the RNeasy mini kit following the manufacturer's instructions (Qiagen, Inc., Valencia, CA, USA). cDNA was synthesized using SuperScript II RNase H-Reverse Transcriptase (Invitrogen; Thermo Fisher Scientific, Inc.). SYBR-Green Master Mix (Applied Biosystems; Thermo Fisher Scientific, Inc.; 10 µl Master Mix, 0.5 µl forward primer, 0.5 µl reverse primer, 1 µl cDNA and 8 µl ddH₂O) was used, and qPCR was performed in accordance with the manufacturer's protocol. The 7000 Sequence Detection system (Applied Biosystems; Thermo Fisher Scientific, Inc.) was applied to perform qPCR analysis. The specific sequences of primers used in the study for gene amplification were shown in Table I. The cycling conditions (33 cycles) were exhibited as followings: 95°C for 5 min, 95°C for 10 sec, 60°C for 30 sec, 95°C for 15 sec, 60°C for 60 sec and 95°C for 15 sec. The expression levels of targeting mRNAs were normalized to that of housekeeping gene of GAPDH using the 2^−ΔΔCq method (20).

Table I.

Primer sequences of RT-PCR test.

Gene	Forward primers (5′-3′)	Reverse primers (5′-3′)
GAPDH C	GGTCCATAGCAAAACGAGG	TACACTACGCAGCCAACACACC
iNOS	TTGGTGGAAGGCAGTTGAGG	CAGCAGGTAGACAAACCATTCA
MCP-5	ATGCCGAGGAACAGATATCTA	CGACCATATCGCACGAGTGCA
TNF-α	AGCACACAAGTGGCACAACG	CATGCGGTCGTAGTCCATAAT
MIP-1α C	AGCAGGCAGCACGTGTCGC	CTTCAACATATGTTAACAGTAC
IL-1β	GAAGTATGCTTAGCCAGTAAG	GAGCGTCGCAATTGTTGTGG
IL-10 C	GATCTGCTATCCCACGGA	CTGACCAGCCATAGCCAGA
SOD1	GGAGCACTGAACGCACAGA	CTACGGAGATTCAAACTCGTG
COX2	CCGCATTCTGGTATAACGAACA	ACCGAGAAGCCAGCACCAT
IL-6	ATTCGGCAACCGAGATATAGA	TGACAACTAGAACGATCCAACC
SOD2	GCATAACTCGAGAACTTACGC	ACTACATTATCGGGTCGGAGTA
CAT	GAGGACTATATCTTCTCGAC	GAATGGTCCCTCGCACTCG
GCLC	GTGACCCTTAACTTGAGAG	AGGACGCAGATCGGACCAACG
Ly6G	GCATCTACGTACAGGACCG	AGTCGGTGATGACAGTATGAG
CD41	ATATCGGCCTATACTCGAT	CAGGATGCTAGTCGTAATGTA

Western blot analysis

The total protein of lung tissue samples and cells was extracted by addition of cold lysis buffer [10 mM Tris-HCl, 1 mM EDTA, and 250 mM sucrose, pH 7.4, containing 15 µg/ml aprotinin, 5 µg/ml leupeptin, 0.1 mM phenylmeth-anesulfonyl fluoride (PMSF), 1 mM NaF, and 1 mM Na₃VO₄ (Beyotime Institute of Biotechnology)] for 50 min at 4°C. Then, the lysates were centrifuged at 12,000 × g for 20 min at 4°C. The soluble protein concentrations in the lysates were assessed using a BCA Protein Assay kit. Next, 40 µg total protein was separated on a 12% SDS-PAGE gel and was transferred onto a polyvinylidene difluoride membrane. Then, the membrane was blocked in 5% dried milk for 2 h at room temperature and was incubated with specific primary antibodies at 4°C overnight. The membrane was then washed with TBS Tween-20 (TBST, containing 0.1% Tween-20) for three times, followed by incubation with a horseradish peroxidase-conjugated secondary antibody (A0208; Beyotime Institute of Biotechnology) at room temperature for 2 h. Following another round of washing with TBST, the membrane was then developed using enhanced chemiluminescence (Thermo Fisher Scientific, Inc.). The antibodies used in the study are shown below. The staining intensity of the bands was quantitated by densitometry through ImageJ software (version 1.49, National Institute of Health, Bethesda, MD, USA). Triplicate experiments with at least triplicate samples were performed. The primary antibodies: Rabbit anti-NLRP3 (1:1,000, cat. no. 15101), rabbit anti-ASC (1:1,000, cat. no. 67824) (both from Cell Signaling Technology, Inc., Danvers, MA, USA), rabbit anti-caspase-1 (1:1,000, ab1872), rabbit anti-Nrf2 (1:1,000, ab31163) (both from Abcam), rabbit anti-HO-1 (1:1,000, cat. no. 70081), rabbit anti-p-ERK1/2 (1:1,000, cat. no. 4370; Cell Signaling Technology, Inc.), rabbit anti-ERK1/2 (1:1,000, ab17942; Abcam), rabbit anti-p-JNK (1:1,000, cat. no. 9255), rabbit anti-JNK (1:1,000, #9252) (both from Cell Signaling Technology, Inc.), rabbit anti-XO (1:1,000, ab109235), rabbit anti-TXNIP (1:1,000, ab188865) (both from Abcam), rabbit anti-p-p38 (1:1,000, cat. no. 9211), rabbit anti-p38 (1:1,000, cat. no. 8690), rabbit anti-p-IKKα (1:1,000, cat. no. 2697), rabbit anti-IKKα (1:1,000, cat. no. 2682) (all from Cell Signaling Technology, Inc.), anti-NF-κB (1:1,000, ab19870), rabbit anti-p-NF-κB (1:1,000, ab86299), rabbit anti-IκBα (1:1,000, ab32518), rabbit anti-p-IκBα (1:1,000, ab24783) (all from Abcam), rabbit and anti-GAPDH (1:500, sc-293335, Santa Cruz Biotechnology, Inc., Dallas, TX, USA). Immunoreactive bands were visualized by ECL Immunoblot Detection system (Pierce; Thermo Fisher Scientific, Inc.) and exposed to Kodak (Rochester, NY, USA) X-ray film. Every protein expression levels will be defined as grey value (ImageJ, Version 1.4.2b, National Institutes of Health) and standardized to housekeeping gene of GAPDH and expressed as a fold of control. All experiments were performed in triplicate and done three times independently.

Statistical analysis

Data are expressed as the means ± standard error of the mean. Treated cells, tissues and the corresponding controls were compared using GraphPad Prism (GraphPad Software, Inc., La Jolla, CA, USA) by a one-way analysis of variance with Dunn's least significant difference tests. P<0.05 was considered to indicate a statistically significant difference.

Results

LR attenuates LPS-induced ALI in mice

Platelets were counted and pulmonary edema was measured with a ratio of lung wet to dry weight. Fig. 1A presents an increased wet/dry ratio in the LPS-treated group and LR reduced this in a dose-dependent manner. In addition, as shown in Table II, PO₂, HCO₃, Hgb, BE and PH increased in the LPS-treated group and these were reduced in LR-pretreated groups. In contrast, LR pretreatment upregulated LAC reduced by LPS but PCO₂ was not significantly different in mice treated as indicated. Arterial blood gas analysis indicated that LR may be protective in LPS-induced ALI in mice. Thromboxane A2 is a marker of platelet activation, and is rapidly hydrolyzed to its inactive stable metabolite, TXB2 (21). Plasma TXB2 were upregulated in mice challenged with LPS and LR treatment dramatically diminished TXB2 expression (Fig. 1B). H&E staining scores were high following LPS treatment indicating lung damage, but this was reversed by LR administration in a dose-dependent manner (Fig. 1C). CD41, a specific platelet marker, can be measured to confirm sequestration of platelets in pulmonary capillaries (22). Platelet activation is involved in ALI (23,24) and immunofluorescence analysis revealed that LR dose-dependently reduced CD41 expression in lung tissues of mice treated with LPS (Fig. 1D). Moreover, RT-qPCR analysis verified downregulated CD41 in LPS-treated lung tissue samples of mice with ALI (Fig. 1E). Thus, LR may have protective effects against LPS-induced ALI.

Figure 1.

LR ameliorates the acute lung injury of mice with LPS induction. (A) The ratio of lung wet to dry weight was measured. (B) TXB2 levels in plasma were evaluated using ELISA method. (C) Representative images of hematoxylin and eosin staining of LPS-induced lung tissues treated with or without LR. Scale bar, 100 µm. (D) The immunofluorescence analysis of CD41 positive levels in lung tissue samples treated under various conditions, and the images were displayed. Scale bar, 100 µm. (E) Reverse transcription-quantitative polymerase chain reaction analysis was used to determine CD41 expression levels in LPS-induced lung tissues of mice administered with different doses of LR. Data are represented as mean ± standard error of the mean of three independent experiments (n=6). ⁺⁺⁺P<0.001 vs. the Con group in the absence of any treatments; ^*P<0.05, ^**P<0.01 and ^***P<0.001 vs. the LPS groups. LPS, lipopolysaccharide; LR, linarin; Con, control; LC-LR, low concentration linarin; MC-LR, medium concentration linarin; HC-LR, high concentration linarin.

Table II.

Blood gas analysis in mice.

Indexes	Con	LPS	LC-LR	MC-LR	HC-LR
PO2 (mmHg)	71.3±1.2	88.9±2.4b	85.1±1.7	80.3±1.9d	78.5±2.2d
PCO2 (mmHg)	37.6±1.3	37.9±1.9	38.1±1.6	38.4±1.5	38.1±1.8
HCO3 (mmol)	16.8±0.4	22.9±1.0a	20.1±0.8	18.6±0.9d	17.8±0.6d
LAC (mM)	3.8±0.2	2.4±0.4b	2.9±0.2d	3.1±0.3d	3.4±0.4e
Hgb (g/dl)	121.81±3.8	148.36±4.2c	135.85±4.8	130.66±4.6d	125.78±2.8e
BE (mEq/l)	−7.6±0.8	−3.3±0.6b	−4.1±0.9	−5.6±1.0d	−6.6±0.8d
PH	7.08±0.02	7.36±0.03a	7.28±0.01	7.13±0.03	7.10±0.04d

PO₂, partial pressure of oxygen; PCO₂, partial pressure of carbon dioxide; HCO₃⁻, bicarbonate level; LAC, lactate concentration; BE, base excess; Hgb, hemoglobin concentration.

^aP<0.05,

^bP<0.01 and

^cP<0.001 vs. the Con group in the absence of any treatments.

^dP<0.05 and

^eP<0.01 vs. the LPS groups.

LR inhibits LPS-induced inflammation infiltration in BALF

BALF cytology data show that alveoli undergo dramatic shifts after ALI (25). BAL total protein calculated as an indicator of lung permeability was elevated after LPS instillation (26). Mice given LR had reduced BAL protein compared to the LPS group (Fig. 2A). BAL cells were increased, indicating lung permeability, was markedly increased by LPS treatment, which was reduced by LR administration (Fig. 2B). In addition, BALF macrophages (MACs), BALF polymorphonuclear leukocytes (PMNs) and lymphocytes were increased with LPS induction. However, LR treatment reduced MACs, PMNs and lymphocytes in BALF (Fig. 2C–E). MPO activity, a marker of neutrophil activation (Fig. 2F) was greater in LPS-treated samples compared to controls. MPO activity was reduced in LR-treated groups.

Figure 2.

LR reduces LPS-induced inflammation infiltration in BALF of mice. (A) Bronchoalveolar lavage protein levels were evaluated. (B) Total BALF cells were evaluated. (C) The number of BALF macrophages (MACs) was measured. (D) The quantification of BALF polymorphonuclear leukocytes (PMNs) was exhibited. (E) The number of BALF lymphocytes was tested. (F) Pulmonary MPO activity was assessed. Data are represented as mean ± standard error of the mean of three independent experiments (n=6). ⁺⁺P<0.01 and ⁺⁺⁺P<0.001 vs. the Con group in the absence of any treatments. ^*P<0.05, ^**P<0.01 and ***P<0.001 vs. the LPS groups. LR, linarin; BALF, bronchoalveolar lavage fluid; MPO, myeloperoxidase; LPS, lipopolysaccharide; Con, control; LC-LR, low concentration linarin; MC-LR, medium concentration linarin; HC-LR, high concentration linarin.

LR inactivates platelets in LPS-induced ALI

Antibodies against leukocyte-specific surface markers of Ly6G, Ly6C and CD11b were used to measure neutrophil-platelet aggregates (NPA) and monocyte-platelet aggregates (MPAs), defined as Ly6G⁺/CD11b⁺/CD41⁺ and Ly6C⁺/CD11b⁺/CD41⁺, respectively. Whole blood extracted from mice had more NPA and MPA after LPS treatment and this was time-dependent. LR (50 mg/kg) considerably reduced the proportion of NPAs and MPAs after LPS-treatment for 48 h (Fig. 3A and B). NPAs in BAL were elevated after LPS induction and then reduced by LR (Fig. 3C). Furthermore, TXB2 in BAL was greater after LPS treatment and this was downregulated by LR dose-dependently (Fig. 3D). High expression of Ly6G induced by LPS was abolished following LR administration (Fig. 3E). Thus, LR can alleviate LPS-induced ALI via inactivating platelets. LPS treatment increased serum and BALF TNF-α, IL-1β, IL-6, MCP-5, MIP-1α COX2 and IL-10 (Fig. 4) and LR administration reduced all of these except IL-10, which was enhanced, indicating an anti-inflammatory effect of LR.

Figure 3.

LR inactivates platelets in LPS-challenged mice with acute lung injury. (A) The percentage of neutrophil-platelet aggregates (NPA) and (B) percentage of monocyte-platelet aggregates (MPAs) in whole blood of mice at different time points after LPS instillation and the effects of LR treatment at described times. (C) NPA quantification and (D) TXB2 levels in BAL were measured. (E) Reverse transcription-quantitative polymerase chain reaction analysis was used to determine Ly6G expression levels in LPS-induced lung tissues of mice administered with different doses of LR. Data are represented as mean ± standard error of the mean of three independent experiments (n=6). ⁺P<0.05, ⁺⁺P<0.01 and ⁺⁺⁺P<0.001 vs. the Con group in the absence of any treatments. ^*P<0.05, ^**P<0.01 and ^***P<0.001 vs. the LPS groups. LR, linarin; LPS, lipopolysaccharide; Con, control; LC-LR, low concentration linarin; MC-LR, medium concentration linarin; HC-LR, high concentration linarin. NPA, neutrophil-platelet aggregates; MPAs, monocyte-platelet aggregates.

Figure 4.

LR reduces LPS-induced pro-inflammatory cytokines release in BALF and serum. TNF-α, IL-1β, IL-6, MCP-5, MIP-1α, IL-10 and COX2 levels in (A) BALF and (B) serum were measured using ELISA methods. Data are represented as mean ± standard error of the mean of three independent experiments (n=6). ⁺⁺P<0.01 and ⁺⁺⁺P<0.001 vs. the Con group in the absence of any treatments. ^*P<0.05, ^**P<0.01 and ^***P<0.001 vs. the LPS groups. LR, linarin; LPS, lipopolysaccharide; BALF, bronchoalveolar lavage fluid; TNF-α, tumor necrosis factor-α; IL, interleukin; MCP-5, monocyte chemotactic protein 5; MIP-1α, macrophage inflammatory protein-1α; COX2, cyclooxygenase 2; Con, control; LC-LR, low concentration linarin; MC-LR, medium concentration linarin; HC-LR, high concentration linarin.

MDA levels induced LPS were reduced after LR treatment (Fig. 5A). In addition, oxidative stress induced by LPS, as evidenced by elevated levels of H₂O₂ and O₂. in lung tissue samples was suppressed by LR treatment, and SOD, CAT and GPx activity in lung tissue samples (Fig. 5B) were elevated by LPS, and LR treatment increased these levels even further suggesting antioxidant activity. RT-qPCR assays demonstrated that SOD2, SOD1, CAT and glutamate-cysteine ligase (GCLC) expression were enhanced with LPS induction and increased more with LR (Fig. 5C). LPS-triggered increased Nrf2 and HO-1 was augmented by LR dose-dependently (Fig. 5D). Thus, LR exerts an antioxidant effect against LPS-induced ALI in vivo.

Figure 5.

LR suppresses oxidative stress induced by LPS in the lung tissues of mice. (A) MDA, H₂O₂ and O₂⁻ levels in the lung tissue samples were calculated. (B) SOD activity, CAT activity, and GPx activity in the lung tissues were measured. (C) Reverse transcription-quantitative polymerase chain reaction analysis of SOD2, SOD1, CAT and glutamate-cysteine ligase (GCLC). (D) Nrf2 and heme oxygenase-1 (HO-1) expression levels were evaluated using western blot analysis. Data are represented as mean ± standard error of the mean of three independent experiments (n=6). ⁺P<0.05, ⁺⁺P<0.01 and ⁺⁺⁺P<0.001 vs. the Con group in the absence of any treatments. ^*P<0.05, ^**P<0.01 and ^***P<0.001 vs. the LPS groups. LR, linarin; LPS, lipopolysaccharide; MDA, malondialdehyde; SOD, superoxide dismutase; CAT, catalase; GPX, glutathione peroxidase; Nrf2, nuclear factor-erythroid 2-related factor 2; Con, control; LC-LR, low concentration linarin; MC-LR, medium concentration linarin; HC-LR, high concentration linarin.

LR inhibits the TXNIP/NLRP3 signaling pathway in the lung tissues of mice exposed to LPS

The TXNIP/NLRP3 signaling pathway is involved in the progression of oxidative stress (27,28). Therefore, immunohistochemical analysis was used to calculate XO and TXNIP in lung tissue samples. Fig. 6A and B show that XO and TXNIP were significantly induced by LPS compared to controls and LR administration reduced expression of XO and TXNIP. Fig. 6C also shows that LR can reduce LPS-induced increased expression of XO and TXNIP. Western blotting indicated that NLRP3, ASC and caspase-1 protein were markedly increased by LPS treatment, and decreased following LR administration (Fig. 6D). Thus, the TXNIP/NLRP3 pathway are involved in LR-modulated ALI induced by LPS.

Figure 6.

LR inactivates TXNIP/NLRP3 signaling pathway in the lung tissues of mice with LPS challenge. (A) xanthine oxidase (XO) and (B) TXNIP expression levels were evaluated through immunohistochemical analysis. The scale bar is 100 µm. (C) The immunoblotting analysis of XO and TXNIP. (D) Western blot analysis was conducted to determine NLRP3, apoptosis-associated speck-like protein containing a C-terminal caspase recruitment domain (ASC) and caspase-1 protein levels in the lung tissue samples of mice treated under various conditions. Data are represented as mean ± standard error of the mean of three independent experiments (n=6). ⁺⁺⁺P<0.001 vs. the Con group in the absence of any treatments. ^**P<0.01 and ^***P<0.001 vs. the LPS groups. LR, linarin; LPS, lipopolysaccharide; XO, xanthine oxidase; Con, control; LC-LR, low concentration linarin; MC-LR, medium concentration linarin; HC-LR, high concentration linarin.

LR impedes MAPK and NF-κB pathways in LPS-exposed mice with ALI

MAPKs (p38-MAPK, ERK1/2-MAPK and JNK-MAPK) are associated with oxidative stress (29). Fig. 7A shows that LPS increased phosphorylated p38, ERK1/2 and JNK, and LR considerably reduced this dose-dependently. Inflammation is key to LPS-induced ALI, so western blotting was used to measure the NF-κB pathway, which is important for regulating the secretion of pro-inflammatory cytokines. Fig. 7B data show that LR reduced LPS-induced phosphorylation of IKK-α, IκBα and NF-κB, indicating LR can be used to reduce inflammation by inactivating the NF-κB signaling pathway.

Figure 7.

LR blocks mitogen-associated protein kinase and NF-κB pathways in LPS-induced mice with ALI. (A) Phosphorylated p38, phosphorylated ERK1/2 and phosphorylated JNK levels were examined by use of western blot analysis. (B) IKK-α, IκBα and NF-κB phosphorylation were tested through western blot analysis. Data are represented as mean ± standard error of the mean of three independent experiments (n=6). ⁺⁺P<0.01 and ⁺⁺⁺P<0.001 vs. the Con group in the absence of any treatments. ^*P<0.05, ^**P<0.01 and ^***P<0.001 vs. the LPS groups. LR, linarin; NF-κB, nuclear factor-κB; ERK, extracellular signal-regulated kinase; JNK, c-Jun N-terminal kinase; IKK-α, IκB kinase-α; Con, control; LC-LR, low concentration linarin; MC-LR, medium concentration linarin; HC-LR, high concentration linarin.

LR reduces inflammation and oxidative stress by suppressing NF-κB and TXNIP/NLRP3 pathways in vitro

LR may be involved in ameliorating LPS-induced ALI in mice. Fig. 8A presents that pro-inflammatory cytokines TNF-α, IL-1β, IL-6, MCP-5, COX2, inducible nitric oxide synthase (iNOS) and MIP-1α were significantly induced by LPS exposure, and in LR-pretreated groups, these cytokines were downregulated in a dose-dependent manner. IL-10 was stimulated by LPS and enhanced by LR. Western blot analysis indicated that LPS exposure stimulated IKK-α, IκBα and NF-κB phosphorylation (Fig. 8B) and LR dose-dependently reduced NF-κB pathway activation. Therefore, LR had an anti-inflammatory role in LPS-induced BEAS-2B cells.

Figure 8.

LR reduces inflammation through suppressing the NF-κB pathway in vitro. The lung epithelia cells of BEAS-2B were pretreated with different concentrations of LR (0, 20, 40 and 80 µM) for 24 h, followed by LPS exposure for another 1 h. Then, all cells were harvested for the following research. (A) TNF-α, IL-1β, IL-6, MCP-5, MIP-1α, IL-10, iNOS and COX2 gene levels in cells treated under various conditions were measured using Reverse transcription-quantitative polymerase chain reaction analysis. (B) IKK-α, IκBα and NF-κB activation were examined via western blot analysis in vitro. Data are represented as mean ± standard error of the mean of three independent experiments (n=6). ⁺P<0.05, ⁺⁺P<0.01 and ⁺⁺⁺P<0.001 vs. the Con group in the absence of any treatments. ^*P<0.05, ^**P<0.01 and ^***P<0.001 vs. the LPS groups. LR, linarin; NF-κB, nuclear factor-κB; LPS, lipopolysaccharide; TNF-α, tumor necrosis factor-α; IL, interleukin; MCP-5, monocyte chemotactic protein 5; MIP-1α, macrophage inflammatory protein-1α; iNOS, inducible nitric oxide synthase; COX2, cyclooxygenase 2; Con, control.

2′-7′-Dichlorofluorescein (DCF) analysis indicated that LPS triggered high production of ROS, which was reduced by LR in a dose-dependent manner (Fig. 9A and B). In addition, in vitro, LR suppressed LPS-triggered high expression of XO and TXNIP (Fig. 9C). In addition, LR reduced NLRP3, ASC and caspase-1 protein expression induced by LPS. Finally, p38, ERK1/2 and JNK phosphorylation were enhanced by LPS treatment, and this was blunted by LR pretreatment in a dose-dependent manner (Fig. 9D).

Figure 9.

LR reduces oxidative stress through suppressing the TXNIP/NLRP3 pathway in LPS-treated cells. The lung epithelia cells of BEAS-2B were pretreated with different concentrations of LR (0, 20, 40 and 80 µM) for 24 h, followed by LPS exposure for 1 h. Then, all cells were harvested for the following research. (A) 2′-7′-Dichlorofluorescein (DCF) analysis was used to calculate ROS generation, and the representative images were displayed. The scale bar is 50 µm. (B) The quantification of ROS production was exhibited. (C) Western blot analysis of XO, TXNIP, LPRP3, apoptosis-associated speck-like protein containing a C-terminal caspase recruitment domain (ASC) and caspase-1 in LPS-treated cells in the presence or absence of LR. (D) p-p38, p-ERK1/2 and p-JNK levels were measured through western blot analysis. Data are represented as mean ± standard error of the mean of three independent experiments (n=6). +++P<0.001 vs. the Con group in the absence of any treatments. ^**P<0.01 and ^***P<0.001 vs. the LPS groups. LR, linarin; LPS, lipopolysaccharide; XO, xanthine oxidase; ERK, extracellular signal-regulated kinase; JNK, c-Jun N-terminal kinase; ROS, reactive oxygen species; Con, control.

Oxidative stress and inflammatory activity of LR depend on ROS production in LPS-treated cells

Fig. 10A indicates that LR reduced LPS- and ATP-induced ROS production compared to LPS- and ATP-single treatment groups. NAC, an ROS scavenger, reduced LPS-induced production of ROS. LR was similar to NAC in suppressing ROS generation. Fig. 10B shows that high expression of XO, TXNIP, p-p38, p-ERK1/2 and p-JNK induced by LPS were downregulated by LR following ATP addition, indicating that reducing oxidative stress-related signaling pathway expression was implicated in LR-ameliorated lung injury. In addition, LR treatment suppressed activation of IKK-α, IκBα and NF-κB in LPS and ATP co-treatment groups (Fig. 10C). Finally, pro-inflammatory cytokines TNF-α, IL-1β, IL-6, MCP-5, COX2, iNOS and MIP-1α were induced by LPS exposure, and this agrees with data in Fig. 8A. Moreover, after ATP addition, the anti-inflammatory role of LR, especially at the highest dose of 40 µM, was observed compared to the LPS group (Fig. 10D). Thus, LR can reduce LPS-induced ROS, inhibiting inflammation and oxidative stress in human lung epithelial cells.

Figure 10.

ROS production is involved in LR-reduced oxidative stress and inflammation in LPS-treated cells. (A) The lung epithelia cells of BEAS-2B were pretreated with LR (80 µM) for 24 h, followed by LPS exposure for another 1 h, and then for addition of 10 mM N-acetylcysteine (NAC) or 5 mM ATP for 0–60 min as indicated. Then, reactive oxygen species production was measured as the relative fluorescence intensity. The lung epithelia cells of BEAS-2B were pretreated with different concentrations of LR (0, 20, 40 and 80 µM) for 24 h, followed by LPS exposure for another 1 h, and then for addition of 5 mM ATP for 60 min. Finally, all cells were harvested for further experiments. (B) XO, TXNIP, p-p38, p-ERK1/2 and p-JNK protein levels were measured using western blot analysis. (C) Western blot analysis of p-IKK-α, p-IκBα and p-NF-κB were exhibited. (D) TNF-α, IL-1β, IL-6, MCP-5, MIP-1α, IL-10, iNOS and COX2 gene levels were evaluated using reverse transcription-quantitative polymerase chain reaction assays. Data are represented as mean ± standard error of the mean of three independent experiments (n=6). ⁺⁺⁺P<0.001 vs. the Con group in the absence of any treatments. ^*P<0.05, and ^**P<0.01 vs. the LPS groups. LR, linarin; LPS, lipopolysaccharide; XO, xanthine oxidase; ERK, extracellular signal-regulated kinase; JNK, c-Jun N-terminal kinase; IKK-α, IκB kinase-α; TNF-α, tumor necrosis factor-α; IL, interleukin; MCP-5, monocyte chemotactic protein 5; MIP-1α, macrophage inflammatory protein-1α; iNOS, inducible nitric oxide synthase; COX2, cyclooxygenase 2; Con, control.

Discussion

ALI is an important cause of significant morbidity and mortality among patients (1,2,30). The lung is continuously exposed to many inhaled infectious agents, and host-derived danger signals (31). Thus, the authors studied LPS-induced ALI in viv and in vitr and identified inflammation and oxidative stress as significant molecular mechanisms contributing to lung injury, findings that support previous research (5,6,32). Notably, LR alleviated LPS-triggered ALI via suppressing the inflammatory response and oxidative stress by inactivating NF-κB and TXNIP/NLRP3 signaling pathways. Therefore, LR alleviates ALI in LPS-induced mice by suppressing inflammation and oxidation.

As previously described, activated platelet function is needed in host defense, affecting the recruitment of lung neutrophils and resulting in the progression of ALI. Platelets become activated at inflammatory sites and adhere to other platelets and leukocytes, forming NPAs or MPAs at exposed endothelia. NPAs are formed in the lung microcirculation and rise in blood and alveolar compartments after injury (33). Thus, circulating leukocyte-platelet aggregates are a marker of platelet activation, and has been reported in patients with inflammatory conditions, such as sepsis, rheumatoid arthritis, coronary diseases, cystic fibrosis, inflammatory bowel disease and acute respiratory distress syndrome (34). Thromboxane A2, an indicator of platelet activation, is rapidly hydrolyzed to the inactive stable metabolite, TXB2 (24). CD41 is a specific platelet marker (23,35). The authors reported that LPS-induced increases in CD41, NPAs, MPAs and TXB2 were downregulated by LR, suggesting that LR treatment could inhibit platelet activation, and perhaps reverse ALI.

Neutrophils and macrophages are chief inflammatory mediators during progression of ALI (36). They infiltrate into lung tissues and release enzymes and phagocytize pathogens. These inflammatory cells are a fundamental source of inflammatory regulators in vivo. In LPS-mediated inflammation, neutrophils and macrophages are activated and recruited to the inflammatory site (37,38). Lymphocytes have also been implicated in the progression of ALI (39,40). In the current study, the authors confirmed that LPS increased these inflammatory cells, evidence of ALI establishment in rodents. Importantly, LR reduced macrophages, neutrophils and lymphocytes to alleviate ALI.

Oversecretion of pro-inflammatory cytokines, including IL-1β, TNF-α, IL-6, MCP-5 and MIP-1α, is key to the inflammatory response (41). Data show that inhibiting multiple inflammatory regulators may attenuate injury in animals (42). Inflammatory cytokines can amplify the inflammatory response by augmenting secretion of chemoattractant factors by airway epithelial cells and alveolar macrophages, as well as through expression of adhesion molecules via epithelial cells and leukocytes (43). Activation of the NF-κB pathway regulated by IKK-α and IκBα is essential for regulating release of pro-inflammatory cytokines (44). In the present study, the authors found that LR possesses anti-inflammatory ability, supported by reduced TNF-α, IL-1β, IL-6, MCP-5 and MIP-1α, and de-phosphorylated IKK-α, IκBα and NF-κB. IL-10, in contrast, is a potent anti-inflammatory molecule and suppresses the action of many pro-inflammatory molecules (45). Consistently, LR enhanced downregulation of IL-10 induced by LPS, confirming its anti-inflammatory capability.

Disturbance of oxidative stress is noted in LPS-induced ALI (46,47). LPS can potentiate XO to generate ROS, including H₂O₂ and O₂⁻ (48). LPS-treatment enhanced XO, elevated H₂O₂, O₂⁻ and MDA, important products of ROS. LR administration decreased XO, H₂O₂ and O₂⁻ SOD, CAT and GPx are major scavengers of ROS, and their activity was decreased in LPS-treated tissues. Constitutive Nrf2 expression is important for sustaining normal redox balance, and it is induced in response to oxidative stress, with subsequent transcription of cytoprotective genes; it is an essential defense against oxidative stress (49). LR induced the expression of Nrf2, and the downstream HO-1 protein in LPS-induced lung tissues, indicating its antioxidant ability. TXNIP binding to NLRP3 has been implicated various diseases (50) and NLRP3 inflammasome activation was observed in ALI (51). In the present study, the NLRP3 inflammasome was activated in LPS-induced tissues and cells, as was its downstream signals of ASC and caspase-1, paralleling IL-1β production and exacerbating lung injury. Furthermore, the TXNIP/NLRP3 signaling pathway has been implicated in oxidative stress (52,53). As previously described, activation of MAPK, including p38, ERK1/2 and JNK, aggravates oxidative stress and injury in lungs (29,54). Then, ROS generation activates MAPK expression (55). In the current study, the authors found that LR administration reduced TXNIP/NLRP3 expression and MAPK phosphorylation in LPS-treated samples. Additionally, ATP treatment combined with LPS in vitr enhanced XO/TXNIP/NLRP3 pathway activity and NF-κB, accelerating cell injury. However, increased ROS induced by ATP in LPS-treated cells were reduced by LR, which down-regulated ROS production. Therefore, LR can suppress lung injury in mice, which might be associated with reduced ROS, subsequently reducing inflammation and oxidative stress.

In conclusion, LPS exacerbated inflammation, oxidative stress and lung injury in mice by activating NF-κB, XO/TXNIP/NLRP3 and MAPK pathways and LR scavenged ROS reduced the inflammatory response and oxidative stress by inhibiting NF-κB, XO/TXNIP/NLRP3 and MAPK pathways. Thus, LR may have promise for treating ALI.

Funding

No funding was received.

Availability of data and materials

All data generated or analyzed during this study are included in this published article.

Authors' contributions

XH and SG made substantial contributions to the conception and design of the present study. XH, YW, MM, QS and HS performed the experiments. XH wrote the paper. SG edited and revised the manuscript critically for important intellectual content. All authors read and approved the manuscript and agree to be accountable for all aspects of the research in ensuring that the accuracy or integrity of any part of the work are appropriately investigated and resolved.

Ethics approval and consent to participate

All experimental protocols were approved by the Institutional Review Board of the Huai'an First People's Hospital, Nanjing Medical University (Nanjing, China).

Patient consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.