Introduction
Excessive, non-specific inflammation in the lungs initiates pathological processes leading to acute lung injury (ALI) and acute respiratory distress syndrome (ARDS), which directly and indirectly cause destruction of lung tissue including alveolar structures [
1]. The development of ARDS is triggered by an immune response that leads to activation of classically activated macrophages, or M1 macrophages, and accumulation of neutrophils in the alveoli. As a result, alveolar epithelial cells and vascular endothelial cells are extensively damaged, and pulmonary edema develops (exudation phase) [
2,
3]. Seven to 10 days after onset, proliferation of type II alveolar epithelial cells and fibroblasts is observed in the destroyed alveoli (proliferative phase) [
1]. This process of reconstruction is accompanied by persistent inflammation can promote alveolar fibrosis and decrease alveolar compliance (fibrotic phase). Alternatively activated macrophages, or M2 macrophages, which differentiate as a result of persistent inflammation, play a key role in promoting disordered alveolar fibrosis [
3]. Overexpression and persistence of M2 macrophages in the alveolar interstitium is a hallmark of the transition to the fibrotic phase [
2,
4]. Therefore, novel therapies to reduce persistent inflammation prior to the establishment of irreversible alveolar fibrosis are required and have attracted great interest.
Molecular hydrogen has potent antioxidant and anti-inflammatory properties [
5,
6]. The mechanisms underlying the anti-inflammatory effects of hydrogen are becoming clearer with known inhibition of proinflammatory cytokines and upstream signaling molecule [
7‐
9]. Previous studies using animal models suggest that hydrogen may ameliorate hyperoxic lung injury, ovalbumin-induced asthma, and anti-type II collagen antibody-induced arthritis (a model for human rheumatoid arthritis) by inhibiting inflammatory signaling by the innate immune system and regulating signaling cascades that impact macrophages [
7,
8,
10]. Inhalation of hydrogen gas may be a straightforward and promising therapeutic option because inhaled gaseous molecules can directly reach the alveoli. Additionally, inhaled hydrogen has a low chemical toxicity [
11,
12]. Thus, this gaseous therapy has good clinical feasibility, as long as its flammability can be controlled.
A recent investigation demonstrated that hydrogen inhalation suppressed increases in oxidative stress and inflammation induced by intratracheal bleomycin administration in mice and suppressed the malignant cycle toward lung fibrosis initiated by transforming growth factor (TGF)-β1 and inflammation [
13]. In the current study, we sought to expand on those findings and assessed lung physiology using basal respiratory function parameters in the same well-established mouse model of ARDS [
14,
15]. Additionally, we examined the upstream mechanisms mediating the protective effects of hydrogen, focusing on macrophage polarization.
Materials and methods
Animals
Eight-week-old, C57BL/6 male mice (21–23 g, specific-pathogen free) were purchased from CLEA Japan Inc (Tokyo, Japan). Mice were kept on a 12-h light/dark cycle at 20 to 22 °C and fed sterile food and water. Every effort was made to minimize the number of experimental animals and minimize pain or distress during the experimental procedures. All protocols followed the principles of laboratory animal care (NIH Publication No. 86-23, revised 1985), and all research protocols were reviewed and approved by the Animal Care and Use Committee, Okayama University (OKU-2018876). This study was conducted in compliance with the ARRIVE guidelines (
https://arriveguidelines.org/). Animal condition was checked twice daily after the administration of bleomycin. Dying animals that met humane endpoint were euthanized by CO
2 asphyxiation and were excluded from the analysis. Before scheduled sampling, animals were sacrificed by exsanguination under deep anesthesia with intraperitoneal administration of 0.75 mg/kg medetomidine hydrochloride (Domitor, Meiji Seika Pharma, Tokyo, Japan), 4 mg/kg midazolam (Dormicum, Astellas Pharma, Tokyo, Japan), and 5 mg/kg butorphanol (Vetorphale, Meiji Seika) as previously described [
16]. All lobes of the right lung were removed
en bloc, snap-frozen using liquid nitrogen, and stored at − 80 °C until use. Then, the right lungs were divided, placed in liquid nitrogen, and ground into a powder. Powdered lung tissue (30 mg) was used for RNA extraction for RT-PCR or protein extraction for Western blot. The left lung was used for histopathological analysis.
Generation of bleomycin-induced lung injury model and inhalation of hydrogen gas
This study was conducted using a well-established mouse model of lung injury and idiopathic pulmonary fibrosis [
15,
17]. In summary, lung injury was generated by administrating bleomycin (bleomycin hydrochloride, Nippon Kayaku, Tokyo, Japan) dissolved in saline intratracheally via tracheotomy [
17]. The bleomycin causes persistent inflammation pharmacologically in the bronchus and alveoli, eventually resulting in alveolar fibrosis. Mice were anesthetized, and an incision was made through the neck into the front of trachea. Bleomycin dissolved in saline (50 µL, 1 mg/kg) was injected using a Hamilton syringe and a 32G needle, then the wound was closed by cyanoacrylate glue. In sham controls, saline without bleomycin was administrated in the same manner. We conducted a preliminary pathologic assessment, which confirmed that bleomycin administration induced lung injury with temporal changes in pathology that mimicked those observed during ALI/ARDS (Additional file
1: Fig. S1).
Mice were randomly assigned to 1 of 4 experimental groups: (1) saline administration and air inhalation (SA group), (2) saline administration and hydrogen inhalation (SH group), (3) bleomycin administration and air inhalation (BA group), and (4) bleomycin administration and hydrogen inhalation (BH group). A gas cylinder containing 4% hydrogen and 96% nitrogen blended gas was prepared (Taiyo Nissan, Tokyo, Japan). By mixing 800 mL/min of the 4% H
2/96% N
2 mixture and 200 mL/min of 100% O
2 gas, a final mixture of 3.2% H
2, 20% O
2 and 76.8% N
2 gas, delivered at 1 L/min, was generated. Air for the control group is created by mixing 800 mL/min of 100% N
2 gas and 200 mL/min of 100% O
2 gas. For gas administration, 5 or fewer mice were placed in a sealed acrylic box (L 40 cm × W 20 cm × H 20 cm) for mixed gas exposure while temperature (acceptable range 22–24 °C) and humidity (acceptable range 40–70%) were monitored. Mice were exposed to either air or 3.2% hydrogen in air for 6 h every day for either 7 or 21 days (Additional file
2: Table S1).
Respiratory physiological examination
The respiratory physiology was evaluated using a FlexVent® small animal ventilator with spirometer (SCIREQ, Montreal, PQ, Canada). The programs for examination of respiratory function were already programmed into the device and were performed according to the manufacturer’s instructions. Mice were anesthetized as described above, and 1 cm of a 18-gauge endotracheal tube was inserted into the trachea by tracheostomy. The endotracheal tube was attached to the FlexVent. Then, mechanical ventilation is started at 150 respirations per minute, 10 mL/kg of tidal volume, and an inspiratory:expiratory ratio of 2:3 for 1 min. Inspiratory capacity (IC) was measured in mL using the “Deep Inflation” program where the lung was inflated with 27 cm H2O of inspiratory pressure. The static compliance (Cst) in mL/cm H2O and the static elastance (Est) in cm H2O/mL were measured using the “PVs-V” program, where the lungs were inflated stepwise with 40 mL/kg of ventilation volume. Cst and Est were calculated by computer analysis according to the pressure–volume (PV) loop curve created. Total respiratory system resistance (Rs) was measured using the “SnapShot-150” program, where 3 repetitions of sine-wave-pressure forced ventilation (1.2 s, 2.5 Hz) were performed. The protocol consisted of 1 min of mechanical ventilation, 1 cycle of deep inflation, and three 1-min cycles of mechanical ventilation using the Deep Inflation, the PVs-V, and finally the SnapShot-150 programs. IC, Cst and Est were calculated as the median of the three individual measurements.
Computed tomography
The lung computed tomography (CT) images were taken using a small-animal CT system, Latheta LCT200® (Hitachi, Ltd. Tokyo. JAPAN). The mice are sedated, then inserted into the CT machine and imaged with the following settings: Imaging condition, lung; Pixel size, 48 μm; Slice thickness, 192 μm; Slice interval, 192 μm; X-ray voltage, Low; Scale of tomographic image, − 700 to + 100; and Respiratory synchronization, “Yes”. Of the 70 slices taken of the whole lung field, 40 slices in the center were used for analysis.
After the CT images were saved as JPG files, images of the inside of the thorax were extracted and converted to 8-bit grayscale. ImageJ (National Institutes of Health, Bethesda, Maryland) was used for subsequent image analysis. To trace the areas in the lung containing air, the “Threshold” program was set at “Range: 0–136”. To measure the area, the following settings in “Analyze Particles” program were used: Size (inch^2), 0 -Infinity; Circularity 0.00–1.00; and Show Bare Outline (the obtained area value was defined as A). When this area value A included components which should be excluded, such as pulmonary vessels, a correction was performed. To calculate the area value of the components to be excluded, the "Threshold" program with Range "137–255" and "Analyze Particles" program with Size (inch^2), 0–Infinity; Circularity 0.00–1.00; Show Bare Outline was used, and the obtained area value was defined as B. The area obtained by subtracting B from A was the true air-containing region. The air-containing capacity of the whole lung field was calculated by integrating the slice width and the area containing air as detected above.
Hematoxylin and eosin and elastica masson staining
The left lung was fixed with 4% paraformaldehyde dissolved in phosphate buffered saline (PBS) for 2 days, embedded in paraffin, then sliced into 4-µm sections. Hematoxylin and eosin (HE) staining and Elastica Masson (EM) staining were performed using standardized protocols by skilled technicians in the Central Research Laboratory at Okayama University. Images were automatically captured using the Nano-Zoomer 2.0RS slide scanner (Hamamatsu Photonics, Shizuoka, Japan) and analyzed using NDP.view2 software, (Hamamatsu Photonics, Shizuoka, Japan). Twenty high-magnification images (total magnification 400×) of HE-stained tissue were captured randomly from one slice, and evaluated using the Lung Injury Score [
18] to quantitate the extent of histologic lung injury and the Ashcroft Score [
19] to quantitate fibrosis.
SYBR Green 2-step real-time reverse transcriptase polymerase chain reaction
Messenger RNA levels for interleukin (IL)-6, IL-4, IL-10, IL-13, collagen type I, fibronectin, and ribosomal protein L4 (RPL4) were assessed using SYBR Green, 2-step, real-time, reverse-transcription PCR. RNA extraction was performed with the Nucleospin
® RNA kit (Takara Bio Inc., Kusatsu, Japan) using powdered lung tissue (30 mg) according to the manufacturer’s instruction. Total RNA (1 μg) was reverse transcribed with ReverTraAce
® qPCR RT Master Mix (TOYOBO Inc., Osaka, Japan). The mixture for SYBR Green PCR was prepared using THUNDERBIRD SYBR qPCR MIX (TOYOBO Inc., Osaka, Japan) and primers (Additional file
2: Table S2). The thermal cycling protocol activated the polymerase for 10 min at 95 °C, followed by 40 cycles of 95 °C for 15 s, and 60 °C for 1 min in a StepOnePlus Realtime PCR machine (Thermo Fisher Scientific, Waltham, Massachusetts).
Bronchoalveolar lavage fluid assays
Bronchoalveolar lavage fluid (BALF) was collected by injecting 1 mL of PBS into the trachea, flushing it in and out 5 times, and then collecting the fluid. After centrifuging at 500 × g at 4 °C, the supernatant was collected, and the total protein concentration was measured via bicinchoninic acid (BCA) assay using the Pierce BCA Protein Assay Kit (Thermo Scientific, Waltham, Massachusetts). Turk's staining solution (200 μL, Nakarai tesque, Kyoto, Japan) was added to the precipitate to stain leukocytes, and the cells were counted using a Burker-Turk counter. To examine IL-6 expression in alveolar macrophages, RT-PCR of BALF cells was performed. Cells were collected by centrifugation from BALF, re-suspended in the lysis buffer included in the Nucleospin XS® RNA kit (Takara Bio Inc., Kusatsu, Japan), and immediately frozen by liquid nitrogen. Then, RNA was extracted according to the manufacturing instructions. The amount of total RNA was 70–100 ng per sample. cDNA was obtained by reverse transcription with ReverTraAce® qPCR RT Master Mix, and real-time PCR for IL-6 was performed.
Western blotting
Powdered frozen graft tissue (30 mg) was mixed with 300 μL of radioimmunoprecipitation assay (RIPA) buffer, which is consisted of 50 mM Tris–HCl (pH 8.0), 150 mM NaCl,1% Igepal® CA-630 (Merck, Darmstadt, Germany), 0.5% Sodium deoxycshoate, 0.1% sodium dodecyl sulfate (SDS) and 1 mM EDTA, and cOmplete™ Mini Protease Inhibitor Cocktail (Merck. Darmstadt, Germany). After homogenizing and measuring the protein concentration, samples were further dissolved in SDS-PAGE sample buffer (62.5 mM Tris–HCl pH 6.8, 10% glycerol, 2% SDS, bromophenol blue) to 1 μg/μL.
For the analysis of collagen type I (COL1), fibronectin and α-smooth muscle actin (αSMA), proteins (10 μg) from lung tissue were separated by electrophoresis on 8% acrylamide gels without SDS and transferred to Immobilon®-P polyvinylidene difluoride (PVDF) membrane (0.45 µm) (Merck, Darmstadt, Germany). For the analysis of TGFβ, proteins (10 μg) from lung tissue were separated by electrophoresis on 12% acrylamide, 0.1% SDS gels.
PVDF membranes are blocked with 5% non-fat dry milk to prevent non-specific binding of antibodies. Primary antibody against fibronectin, αSMA, COL1, and TGFβ were diluted with Can Get Signal immunoreaction enhancer solution 1 (Toyobo, Osaka, Japan) (Additional file
2: Table S3), and incubated with the membranes overnight at 4 °C. Horseradish-peroxidase–conjugated secondary antibodies against mouse IgG and rabbit IgG were diluted with Can Get Signal immunoreaction enhancer solution 2 (Toyobo, Osaka, Japan) and membranes were incubated for 2 h at room temperature. Chemiluminescence detection was performed with ECL Prime Western Blotting Detection Reagents (Cytiva, Tokyo, Japan) and a WSE-6100 LuminoGraph I (ATTO Corporation, Tokyo, Japan).
Immunohistochemistry
Paraffin-embedded lung tissue sections (4 µm) were immunostained for TGF-β and IL-6 using an ABC Kit (Vector laboratories INC., Burlingame, California). Information on the primary and secondary antibodies used is provided in Additional file
2: Table S3. Sections were deparaffinized, rehydrated, and treated for antigen retrieval with 10 mM citric acid pH 6.0 at 120 °C for 10 min in a pressure cooker. Endogenous peroxidase inhibition was performed with 0.3% hydrogen peroxide in PBS for 20 min at room temperature. Blocking treatment was performed with 10% goat serum in tris buffered saline with 0.1% Tween 20 (TBS-T) to prevent non-specific binding of antibodies. The primary antibodies were diluted by Can Get Signal immunostaining Solution A (Toyobo, Osaka, Japan), applied to the sections, incubated overnight at 4 °C, and then washed with TBS-T. Biotin-conjugated secondary antibodies were diluted by Can Get Signal immunostaining Solution A, applied on the sections, and incubated for 2 h at room temperature. After washing, ABC reagent was applied to the sections then incubated for 30 min at room temperature as per the manufacturer’s instructions. For 3,3′-diaminobenzidine (DAB) staining, one DAB tablet (10 mg per tablet, FUJIFILM Wako Pure Chemical Corporation, Osaka, Japan) was dissolved in 50 mL of 0.05 mol/L Tris–HCl buffer pH 7.6 with 10 μL of 30% hydrogen peroxide as per the manufacturer’s instructions. Sections were incubated in DAB solution for 10 min at room temperature, then washed under running water, counterstained with hematoxylin, dehydration, clearing, and coverslipping.
Immunofluorescence
Paraffin blocks were sectioned, deparaffinized, rehydrated, and treated for antigen retrieval using the technique described above. The multiplex fluorescent immunostaining was used for staining with anti-ionized calcium binding adaptor molecule 1 (Iba-1) antibody and anti-CD163 antibody. Information on primary and secondary antibodies is provided (Additional file
2: Table S3). Blocking treatment was performed with Super Block
® (SCY AAA125, Cosmo Bio Co., Ltd. Tokyo, Japan). Anti-Iba-1 antibody and anti-CD163 antibody were diluted in Can Get Signal immunostaining Solution A, then incubated on the tissue section overnight at 4 °C. After washing, the sections were incubated with fluorescently labeled secondary antibodies with Alexa Flour (AF) 488 or 594. DAPI-Fluoromount G
® (0100-20, SouthernBiotech, Birmingham, AL) was used for nuclear staining and sealing.
Fluorescent images were taken by the Mantra™ Quantitative Pathology Imaging System (PerkinElmer Inc., Waltham, Massachusetts), and cells were counted in the alveoli and interstitium were automatically using the InForm® 2.4.10 software (Akoya Biosciences, Inc., Menlo Park, California). Three images were taken randomly from each section with a 200× image. Fluorescence imaging was performed at 488 nm, and 594 nm wavelengths. In the InForm software, a computer learning system was used to learn the characteristics of alveolar epithelium and alveolar interstitum tissues and exclude tracheal epithelial cells. The cells were identified by DAPI staining, and the immunostaining was visualized at 488 nm (Iba-1) or 594 nm (CD163) wavelength. The intensity thresholds for Iba-1-positive and CD163-positive cells were carefully adjusted and identified, and all images were analyzed according to the same rules.
Statistics
Statistical analysis was performed using IBM SPSS Statistics version 23.0 (IBM, Armonk, New York). Statistically significant differences between groups were determined using an unpaired two-tailed Student’s t-test for single comparisons; the Kruskal–Wallis test followed by Dunn's multiple comparison test for multiple comparisons. All values are presented as mean ± 95% confidence interval (CI). Results were considered significant at p < 0.05.
Discussion
Hydrogen inhalation therapy has been proven effective in mitigating in several animal models of lung injury including hyperoxic lung injury, hemorrhagic shock-induced lung injury, radiation-induced lung injury, and bronchial asthma [
7,
8,
20,
21]. Our study is the first to prove that hydrogen inhalation therapy effectively attenuates the decline of respiratory physiological function induced by bleomycin in a mouse model of persistent lung inflammation and fibrosis. To the best of our knowledge, this is the first study to assess the effects of hydrogen inhalation using physiologic respiratory function tests and CT volumetry. We also demonstrated that the protective effects of hydrogen gas inhalation therapy in this lung injury model were accompanied by attenuation of pro-inflammatory cytokine expression and reduced the number of M2-biased macrophages in the lung after bleomycin-induced lung injury).
In this study, we administered an air mixture with 3.2% hydrogen for 6 h daily beginning on the day of bleomycin administration and continuing for 21 days. Other investigations of inhaled hydrogen therapy have shown effective results with hydrogen concentrations of 2–4% [
5,
7,
20‐
24], and repeated inhalation was reported to be more effective than continuous inhalation in rat model of Parkinson’s disease [
25]. Because the endpoint of this study was to assess lung function during the fibrotic phase after lung injury, we targeted treatment during the proliferative phase of ARDS, which ordinary occurs 7 to 21 days after the onset of lung injury [
1]. Our preliminary studies indicated that the bleomycin-induced lung injury model mimicked the temporal changes in pathology observed during ARDS and dictated our protocol of repeated hydrogen inhalation for 21 days after bleomycin administration.
During ARDS, pathogen-associated molecular pattern molecules and damage-associated molecular pattern molecules stimulate type II alveolar epithelial cells and alveolar macrophages to secrete pro-inflammatory cytokines. The permeability of pulmonary capillaries and alveolar epithelial cells increases, and exudate flows from the blood vessels into the alveoli and interstitium. The immune cells responsible for this are classically activated macrophages (M1 macrophages) and neutrophils [
1]. IL-6, which is expressed in type II alveolar epithelial cells and M1 macrophages, is associated with lung fibrosis through the polarization of M2 macrophages [
26‐
30]. Although M2 macrophages are important for tissue repair, an excess of M2 macrophages can cause organ fibrosis [
31,
32]. Suppression or deletion of IL-6 suppresses M2 macrophage polarization and attenuates lung fibrosis [
33,
34]. In our study, immunostaining showed the expression of IL-6 was induced in alveolar macrophages by bleomycin administration. Although it is difficult to differentiate between the IL-6 produced by the cells and that bound to cells, IL-6 was most likely secreted by alveolar cells considering upregulation of IL-6 in BALF cells. Our finding that hydrogen inhalation therapy reduced IL-6 mRNA expression is consistent with published work demonstrating that hydrogen suppresses the expression of IL-6 [
7,
20,
35‐
41]. Therefore, it is reasonable to speculate that the reduction in IL-6 expression in response to hydrogen inhalation therapy caused less M2-biased macrophage polarization and less fibrosis after bleomycin-induced lung injury.
IL-4 and IL-13 also induce the polarization of macrophages to M2 macrophages, which decreases inflammation and encourages tissue repair. Persistent or excessive expression of IL-4 or IL-13 and the accompanying M2 macrophage polarization leads to abnormal organ fibrosis [
31,
32]. In our study, the expression of IL-4 and IL-13 mRNAs were decreased by hydrogen inhalation therapy. The regulation of IL-4 and IL-13 by hydrogen may result in an anti-fibrotic effect through suppression of M2-biased macrophage polarization and thereby reduce alveolar fibrosis. TGF-β is secreted from M2 macrophages [
42]. Hydrogen administration decreased the number of TGF-β-positive cells in the alveolar interstitium, again indicating that control of M2-biased macrophage polarization may be an important mechanism underlying the therapeutic benefits of inhaled hydrogen. However, as another interpretation, the decrease in TGF-β1 positive cells by immunostaining could also be the result of downregulation of TGF-β1 production in mesenchymal cells and/or epithelial cells by hydrogen gas inhalation, reflected in the decrease in TGF-β1 binding to TGF-β1 receptors on macrophages in the interstitum. The results of this study support models put forth by others that hydrogen therapy regulates upstream signals in a cascade impacting macrophages and innate immunity that leads to inflammation [
7,
8,
10,
43].
The study has some limitations. The pathogenesis of lung injury in clinical practice is diverse. Bleomycin-induced lung injury is only one type of drug-induced lung injury and does not replicate all possible lung injury presentations. Second, determining the most effective hydrogen administration regimen—timing, duration and concentration—will be required for clinical application. Third, to identify M2-biased macrophages by immunostaining, we used anti-CD163 antibody, although the expression of CD163 antigen does not necessarily associate with the entire cellular phenotype of M2 macrophage [
44]. Finally, the mechanisms by which hydrogen inhibits bleomycin-induced lung injury were not fully elucidated in this study. Hydrogen reduced the number of M2-biased macrophages in the alveolar interstitium with associated inhibition of increases in IL-6, IL-4 and IL-13 that occur after lung injury. Although we observed a convincing impact on M2-biased macrophages in response to hydrogen, currently, we do not have clear evidence that hydrogen directly affects macrophage polarization or fibrotic potential. Moreover, the classification of polarized macrophages is rather complex, and M2 macrophages are divided into subclasses. A study to determine the effects of hydrogen on macrophage polarization, fibrotic potential, or M2 macrophage subclass as a potential underlying mechanism of hydrogen therapy is warranted and may advance our understanding of hydrogen biology.
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