Blood purification is an emerging approach to dampening the cytokine storm. This study aims to assess the efficacy of HA330 resin-directed hemoadsorption (HA) on endotoxin-induced porcine acute respiratory distress syndrome (ARDS) model.
Methods
Twenty-four Chinese domestic pigs were allocated into saline group receiving intravenous infusion of saline (N = 6) and endotoxin group receiving intravenous infusion of LPS (N = 18). When ALI model was initially diagnosed, six pigs in the LPS and saline group were killed for BALF and histopathological analysis. The remaining 12 pigs in LPS group received 3-h HA (N = 6) or HA-sham (N = 6) treatment, respectively. Following another 5-h observation, animals were killed. Variables on hemodynamics, blood gases and lung mechanics were recorded at a series of time points. Differentially expressed cytokines and proteins were determined by ELISA and proteomics.
Results
HA treatment significantly improved injured oxygenation induced by LPS. HA also partially improved the barrier permeability and reduced lung edema and inflammation/injury induced by LPS infusion. Proteomic analysis showed the differentially expressed proteins between HA- and HA-sham-treated groups mostly belonged to the categories of acute inflammation/immune response, and proteolysis.
Conclusions
Hemoadsorption improved ARDS possibly by blunting the cytokine storm and by restoring homeostasis of the disordered proteome milieu in the exudative phase.
The acute respiratory distress syndrome (ARDS) is a condition with the acute onset of noncardiac respiratory failure that develops in response to a series of insults to the alveolar-capillary barrier [1]. The current mainstay therapy for ARDS is largely supportive [2, 3]. This has been shown to reduce mortality by limiting further iatrogenic injury to the already injured lungs. However, the mortality rate of ARDS is still unacceptably high [4]. ARDS is largely caused by the local alveolar and circulating “cytokine storm” that happens with bacterial/virus infection, burn/trauma and some possible iatrogenic factors, such as high-volume ventilation [5]. This has encouraged the development of several specific targeted pharmacologic therapy directed against single key pathogenic mediators. However, most clinical trials have proven no benefit to disease outcome and were stopped early for futility [6]. Investigators shifted their interests into the extracorporeal blood purification (EBP) modality, which is a nonspecific, broad-spectrum method to blunt the “cytokine storm” by immediately clearing a series of circulating and resident mediators [7].
Until now, there are only some inconsistent preliminary data to investigate the effects of hemofiltration (a modality of EBP) on ARDS animal models [8, 9]. Also, it has been shown that hemoadsorption (HA), another modality of EBP, can improve oxygenation in septic patients [10, 11]. However, evidences of HA’s effects on ARDS patients animal models are scarce. We hypothesize that HA can improve oxygenation, reduce the permeability of alveolar-capillary barrier and alleviate pulmonary edema/damage by blunting the circulating/alveolar cytokines in the process of ARDS. To test this hypothesis, we established an endotoxin-induced ARDS porcine model to explore HA’s therapeutic effect by using a HA330 resin cartridge (a new weapon against cytokine storm).
Methods
Research animals and ethical considerations
This study was approved by the Institutional Animal Experiment Committee of Beijing Hospital. All experiments were performed according to the Declaration of Helsinki conventions for the use and care of animals. Twenty-four healthy, 3–4-week-old Chinese domestic white pigs of both sexes were chosen from a local stock routinely used for the experimental research. The average weight of pigs used in this experimental procedure is 43 ± 0.3 kg (mean ± SEM).
Animal preparations
Sedation, anesthesia and muscle relaxation
Detailed information is shown in Additional file 1: Supplement-Methods.
Ventilation and measurements of lung mechanics
Animals were ventilated in a volume-controlled mode. The ventilation protocol at baseline used a tidal volume of 10 ml/kg body weight, a fraction of inspired oxygen (FiO2) of 0.4 and a positive end-expiratory pressure (PEEP) at 0 cmH2O. Parameters of lung mechanics were recorded. Detailed information is shown in Additional file 1: Supplement-Methods.
Instrumentation and hemodynamic measurements
Cardiac output (CO), mean arterial pressure (MAP), systematic vascular resistance (SVR), mean pulmonary arterial pressure (MPAP), pulmonary vascular resistance (PVR), pulmonary artery wedge pressure (PAWP), extravascular lung water (EVLW) and pulmonary vascular permeability index (PVPI) were measured with PiCCO and Swan-Ganz systems. Detailed information is shown in Additional file 1: Supplement-Methods.
Experimental protocol
After surgical preparations and instrumentation, all animals were ventilated in prone position and a period of 1 h was left for animal stabilization. Thereafter, baseline (i.e., the time point after 1-h stabilization) parameters including lung mechanics, hemodynamics, blood gases were recorded and venous blood samples were collected. As a next step, lung injury model was produced with i.v. infusion of 50 μg/kg LPS (Escherichia coli, serotype O55:B5, Sigma-Aldrich, St. Louis, MO, USA) mixed in 500 ml of saline that was delivered via a volumetric infusion pump (Instrumentation Laboratory, Bedford, MA, USA) for about 2 h [12, 13]. Before the start of the experiment, 24 animals were purchased and randomly divided into four groups according to different conditions: (a) control group (N = 6), animals received an i.v. infusion of saline without LPS (LPS-sham); (b) LPS group (N = 6), animals received an i.v. infusion of saline with LPS as indicated above. When experimental ARDS was diagnosed in LPS group (PaO2/FiO2 is equal or less than 200 mmHg with a PEEP equal to 5 cmH2O), animals in control and LPS group were all killed for bronchoalveolar lavage fluid (BALF) and histologic assessment in order to aid further diagnosis of lung injury. (c) LPS plus HA-sham group (N = 6), animals received an i.v. infusion of saline with LPS. Immediately after ARDS was well established, HA-sham treatment was started by using a hollow fiber membrane hemofilter (Fresenius) with the ultrafiltration line clamped. Two animals in this group were excluded because they died or developed severe sepsis/septic shock and refractory acidosis despite active liquid recovery and vasopressor administration before moderate ARDS diagnosis; (d) LPS plus HA group (N = 6), animals received an i.v. infusion of saline with LPS, and real HA treatment was started by using a disposable hemoperfusion cartridge (HA330 resin, styrene divinylbenzene copolymers, with a blood flow of 200–250 ml/min, volume of 185 ml; Jafron Biomedical Co., Ltd., Zhuhai, GuangDong, China; http://www.jafron.com/). Two pigs were also discarded because they died of septic shock and severe disturbance of water, electrolyte and acid base before the establishment of hemoperfusion circulation. HA-sham and HA treatment lasted for 3 h, and thereafter, the animals were monitored for an extended observation period of 5 h and then killed with a bolus injection of 10 ml of 15% KCl. BAL fluid collection and lung tissue harvesting were performed immediately upon exsanguination and sternotomy performance for the measurements of inflammatory markers, proteomes and for histologic evaluation. Parameters of hemodynamics, blood gases and lung mechanics were recorded every hour following the start of LPS or sham LPS infusion until the end of experiment. Plasma samples were also prepared in the corresponding time points. During the experiment, all pigs were continuously infused with Ringer lactate solution or saline at a rate of 12 ml/kg/h at the start of the experiment. The infusion rate was increased to 15–20 ml/kg/h if the MAP was less than 70–50 mmHg. However, if pulmonary artery wedge pressure (PAWP) continuously raised and exceeded 12 mmHg, the rate of infusion should be reduced to prevent fluid overload. Meanwhile, norepinephrine (0.5–1.5 μg/kg/min) was then used to achieve this level of mPAP in LPS-treated pigs. Body temperature was maintained over 36 °C by using a heating blanket. The experimental protocol was summarized in Additional file 2: Fig. S1.
Assessment of the LPS-induced ARDS porcine model
To determine whether ARDS has occurred, at least four main features of ARDS should be assessed: (1) abnormalities of gas exchange. A ratio of the partial pressure of arterial oxygen to the fraction of inspired oxygen (PaO2/FiO2) ≤ 200 mmHg at PEEP = 5 cmH2O (clinical diagnostic criteria of moderate ARDS) is the initial evaluating criteria;(2)a remarkable leakage of alveolar barrier as indicated by the significant increase of lung wet-to-dry weight ratio, EWLW and PVPI; (3) a significant infiltration of inflammatory cells and production of inflammatory cytokines in both circulation and lung tissues (plasma and lung IL-6, IL-8, IL-1β, IL-17A and TNF-α levels were measured in our study); (4) diffuse alveolar damage (DAD) as determined by lung histopathological examination [14].
HA330 cartridge-directed hemoadsorption
The HA330 is an electrically neutral microporous resin that is a powerful new weapon in the clearance of “cytokine storm” occurred in sepsis [10]. Detailed information is shown in Additional file 1: Supplement-Methods.
BALF recovery
Sixty milliliter ice-cold saline was used to collect BALF in the left upper, middle and lower lobes. Detailed information is shown in Additional file 1: Supplement-Methods.
Assessment of total protein contents in BALF
BCA (bicinchoninic acid) protein assay reagent kit (Pierce Biotechnology, Rockford, IL, USA) was used. Detailed information is shown in Additional file 1: Supplement-Methods.
Lung tissue collection and histopathological evaluation
The right lower lobe was excised, fixed and sliced for routine hematoxylin and eosin (H&E) staining. ALI scoring was done according to a consensus report published previously [14] (Additional file 3: Table S1). Detailed information is shown in Additional file 1: Supplement-Methods.
Lung water assessed by gravimetric method
Samples from unused right lung lobes were dissected free of non-lung parenchymal tissue, placed in a dish and weighed (wet weight). Then, they were dried in an oven at 80 °C and weighed daily until their weight was maintained unchanged (dry weight). The total water content of the lung was crudely estimated as a wet-to-dry weight ratio (W/D).
Concentrations of proinflammatory mediators in circulation and lung tissues
IL-1β, IL-6, IL-8, TNF-α and IL-17A were measured by ELISA kits (Bluegene Biotech CO., LTD, Shanghai, China). Detailed information is shown in Additional file 1: Supplement-Methods.
Plasma and lung proteome
Protein samples of plasma, BALF and lung tissue in HA or HA-sham treatment group were collected and received iTRAQ-labeled (Applied Biosystems, Foster City, CA, USA) mass spectrometric analysis. Bioinformatics analysis was also performed [15, 16]. Detailed information is shown in Additional file 1: Supplement-Methods.
Statistical analysis
The data are shown as the mean ± SEM. Parametric data between multiple groups were compared by using the Kruskal–Wallis test and followed by Mann–Whitney U test if statistically significant. Mann–Whitney U test was also used for the comparison between two independent continuous variables. Data were analyzed using the SPSS statistical software package for Windows, version 13.0 (SPSS, Chicago, IL, USA), and P < 0.05 was considered as statistically significant.
Results
Intravenous infusion of endotoxin causes sharp changes in physiological parameters
The ratio of PaO2/FiO2 and alveolar-arterial oxygen partial pressure difference (AaDO2) in pigs that received LPS infusion declined gradually (from 440 ± 19 to 157 ± 23 mmHg, P < 0.001, Fig. 1a; Table 1). After LPS infusion, CO was firstly increased and then decreased when moderate ARDS was diagnosed. However, the changes did not reach statistical difference when compared with saline group. LPS infusion increased MPAP (18.8 ± 1.5 vs. 41.0 ± 1.7 mmHg, P < 0.001, Fig. 1b; Table 2) and PVRI (201 ± 13 vs. 781 ± 74 dyn s/cm5/m2, P < 0.001, Table 2). However, MAP and SVRI continued to decrease (Table 2). In addition, pulmonary mechanics were also damaged as shown by an increase in PAWPeak, PAWPlateau and resistance and a decrease in pulmonary static compliance (Fig. 1c, d; Table 1).
Fig. 1
LPS impairs lung function and alveolar-capillary barriers. Pigs were allocated into intravenous saline and LPS group, respectively. Parameters of oxygenation, hemodynamics and lung mechanics were recorded at different time points from baseline to the end of the experiment (T0). BALF and lung tissues were collected at T0. PaO2/FiO2 (a) was measured by using blood samples from femoral artery on a blood gas analysis instrument. The value of mPAP (b) was gained by Swan-Ganz catheter implantation into jugular vein. Compliance (c) and resistance (d) were recorded by using Drager Evita 4 ventilator. EVLWI (e) and PVPI (f) were measured by PiCCO system at baseline and a series of time points until ALI was well established (T0). g Whole protein content in the BALF of pigs was detected by using BCA protein assay kit. h The ratio of wet/dry lung weight of saline control and LPS challenge pigs. i Whole-cell counts in the BALF collected from both groups of pigs. j and k were the representative histology sections of controls and LPS challenge pigs. HE sections are from one representative animal per group. l Lung injury scores were calculated according to ATS report which was in detail described in the “Methods.” Data points are expressed as mean ± SEM, N = 6 of each group. Statistical significance between saline and LPS group per point of measurement is shown as *P < 0.05; **P < 0.01; ***P < 0.001, respectively
Table 1
Variables determining oxygenation and lung mechanics in saline controls and LPS-challenged animals
Parameter
Group
Time (h)
Baseline
−3 h
−2 h
−1 h
T0
PaO2/FiO2 (mmHg)
NS
466 ± 26
458 ± 60
531 ± 51
509 ± 60
479 ± 34
LPS
440 ± 19
312 ± 51
242 ± 36***
194 ± 10***
157 ± 23***
PaCO2 (mmHg)
NS
35.2 ± 2.8
30.8 ± 2.8
30.5 ± 1.8
32.3 ± 1.1
31.8 ± 1.49
LPS
36.8 ± 2.4
30.2 ± 1.8
37.5 ± 1.5
36.5 ± 3.0
44.7 ± 5.0**
AaDO2 (mmHg)
NS
47 ± 7
48 ± 14
52 ± 1
51 ± 12
60 ± 4
LPS
63 ± 5
124 ± 20
143 ± 15**
213 ± 53**
224 ± 48**
PAWPeak (mbar)
NS
16.5 ± 1.8
16.5 ± 1.5
16.5 ± 1.7
17.3 ± 2.0
17.3 ± 1.8
LPS
21.3 ± 0.9
27.2 ± 1.8**
30.2 ± 2.4***
31.2 ± 2.4***
35.7 ± 2.5***
PAWPlateau (mbar)
NS
12.2 ± 1.8
11.5 ± 1.7
12.2 ± 2.0
13.2 ± 2.3
13.8 ± 2.2
LPS
15.3 ± 1.2
18.8 ± 1.4
22.3 ± 2.3**
25.7 ± 2.5***
27.3 ± 3.2***
Resistance (mbar/l/s)
NS
9.3 ± 1.4
7.9 ± 1.2
8.1 ± 1.3
7.5 ± 1.1
8.1 ± 1.3
LPS
8.5 ± 0.4
13.6 ± 2.5
15.7 ± 3.5
15.1 ± 3.2
14.7 ± 2.2
Compliance (ml/mbar)
NS
31.2 ± 3.5
33.3 ± 3.0
34.5 ± 4.0
35.6 ± 4.3
32.8 ± 3.3
LPS
28.2 ± 2.7
23.0 ± 2.1
21.4 ± 2.3*
20.7 ± 2.9**
16.7 ± 1.8**
Oxygenation and ventilation parameters in saline control and LPS challenge animals at baseline and a series of time points until the end of the experiment when ALI model was diagnosed (data shown are mean ± SEM, N = 6 of each group; *P < 0.05; **P < 0.01; ***P < 0.001 versus control group). PaO2, oxygen partial pressure; FiO2, inspiratory oxygen fraction; PaCO2, carbon dioxide partial pressure; PAWPeak, peak airway pressure; PAWPlateau, plateau airway pressure
Table 2
Systemic and pulmonary hemodynamic measurements in saline controls and LPS-challenged animals
Parameter
Group
Time (h)
Baseline
−3 h
−2 h
−1 h
T0
CO (l/min)
NS
4.1 ± 0.3
4.5 ± 0.4
4.1 ± 0.4
4.2 ± 0.4
4.2 ± 0.4
LPS
4.1 ± 0.3
4.1 ± 0.5
5.1 ± 0.3
5.0 ± 0.3
3.4 ± 0.3
MAP (mmHg)
NS
105 ± 6
98 ± 6
102 ± 8
101 ± 7
102 ± 8
LPS
113 ± 3
78 ± 8
56 ± 4***
57 ± 5***
54 ± 5***
SVRI (dyn s/cm5/m2)
NS
1783 ± 198
1810 ± 169
1927 ± 148
1822 ± 183
1909 ± 218
LPS
2399 ± 238
1987 ± 217
1002 ± 111**
952 ± 56**
1160 ± 97*
mPAP (mmHg)
NS
16.5 ± 1.0
16.7 ± 0.5
15.7 ± 1.2
17.8 ± 1.5
18.5 ± 1.2
LPS
18.8 ± 1.5
28.8 ± 1.9***
3.3 ± 2.0***
34.7 ± 2.7***
41.0 ± 1.7***
PVRI (dyn s/cm5/m2)
NS
204 ± 20
193 ± 16
231 ± 48
209 ± 35
201 ± 13
LPS
364 ± 40
552 ± 115***
542 ± 67**
634 ± 120***
781 ± 74***
PAWP (mmHg)
NS
6.0 ± 1.2
6.5 ± 1.5
6.3 ± 1.4
6.8 ± 1.5
6.8 ± 1.2
LPS
4.0 ± 1.2
5.5 ± 0.6
8.0 ± 0.6
9.0 ± 0.9
12.2 ± 1.4*
EVLWI (ml/kg)
NS
9.0 ± 0.5
9.7 ± 0.9
9.3 ± 0.5
9.5 ± 0.6
10.0 ± 0.9
LPS
8.0 ± 0.5
9.7 ± 0.7
9.8 ± 0.9
11.0 ± 0.8
15.4 ± 1.3***
PVPI
NS
2.7 ± 0.1
2.8 ± 0.3
3.0 ± 0.3
3.0 ± 0.3
2.9 ± 0.2
LPS
2.7 ± 0.2
3.6 ± 0.3
4.0 ± 0.7
4.6 ± 0.7
5.6 ± 0.5***
Hemodynamic parameters are compared between the saline control and LPS-challenged group. (Data are mean ± SEM, N = 6 of each group; *P < 0.05, **P < 0.01, ***P < 0.001; versus control group)
CO cardiac output, MAP mean arterial pressure, SVRI systemic vascular resistance index, MPAP mean pulmonary arterial pressure, PVRI pulmonary vascular resistance index, PAWP pulmonary artery wedge pressure, EVLWI extravascular lung water index, PVPI pulmonary vascular permeability index
Intravenous infusion of endotoxin causes high-permeability pulmonary edema and lung histologic damages
The EVLWI continuously increased after LPS infusion until ARDS was diagnosed (from 8.0 ± 0.5 ml/kg in baseline to 15.4 ± 1.3 ml/kg at the end of this experiment when ARDS was established, P < 0.001; Fig. 1e). In parallel, there was also a remarkable increase in lung wet/dry ratio in LPS-challenged pigs compared with saline group (Fig. 1h). The alveolar-capillary membrane was also seriously injured by LPS infusion as manifested by a significant increase in both pulmonary vascular permeability index (PVPI) and whole BAL protein concentration (Fig. 1f, g). Infusion of LPS in the endotoxin challenge group was also associated with an increase in the numbers of whole BAL cell counting (Fig. 1i). To determine the histopathological features of ALI model, subset of animals (N = 6 in LPS and saline group, respectively) were killed when ARDS model was diagnosed based on oxygenation parameter (PaO2/FiO2 ≤ 200 mmHg at PEEP = 5 cmH2O). Histologic examinations from animals receiving LPS demonstrated alveolar bleeding, microatelectasis, perivascular edema, marked leukocyte sequestration in alveolar septa and lumen, thickened alveolar walls, and the presence of proteinaceous debris in the alveolar space as compared to control subjects (Fig. 1j–l, Additional file 4: Fig. S2).
Intravenous infusion of endotoxin augments the expressions of systemic and pulmonary inflammatory cytokines
As shown by ELSA assay in Fig. 2, there was no difference in the baseline concentration of plasma IL-1β (Fig. 2a), IL-6 (Fig. 2d), IL-8 (Fig. 2g), TNF-α (Fig. 2j) and IL-17A (Fig. 2m) between LPS and saline groups, but all of these cytokines increased rapidly when challenged with LPS infusion at T0 compared with saline infusion. We also determined the levels of these inflammatory cytokines within BALF and lung homogenates to assess the inflammatory response in the alveolar compartment. ELISA assay showed significant increased levels of these cytokines in BALF and lung homogenates after LPS challenge except IL-17A, which was remarkable increased in BALF but remained unchanged in lung homogenates at T0 (Fig. 2).
Fig. 2
Concentrations of circulating and pulmonary inflammatory parameters. In LPS group, plasma samples were collected before LPS challenge (baseline) and at the time when ARDS model had been well established (T0). BALF and lung homogenates were also prepared at necropsy. Samples from saline control group were also obtained at the corresponding time points. The level of circulating and pulmonary IL-1β (a–c), IL-6 (d–f), IL-8 (g–i), TNF-α (j–l) and IL-17A (m–o) was detected by using commercial ELISA kits. Data are presented as mean ± SEM (N = 6 of each group). Compared with saline (NS) group, *P < 0.05; **P < 0.01; ***P < 0.001
Hemoadsorption improves oxygenation and lung mechanics in pigs challenged with endotoxin
We found that treatment with HA increased LPS-impaired oxygenation (387 ± 10 mmHg at baseline vs. 183 ± 6 mmHg at T0 vs 315 ± 22 mmHg at 8 h after HA; Fig. 3a; Table 3). In contrast, in endotoxin-challenged pigs that did not receive HA (HA-sham) treatment, the ratio of PaO2/FiO2 was only slightly increased at 8 h after HA-sham (Fig. 3a; Table 3). Treatment with HA significantly or showed a trend toward decreasing PAWPeak, PAWPlateau, lung resistance and the impairment of static compliance induced by endotoxin infusion when all pigs data were pooled together and compared with HA-sham group (Fig. 3c, d; Table 3). However, HA did not alter the impairment of systemic/pulmonary hemodynamic parameters (Fig. 3b; Table 4).
Fig. 3
Effects of HA on oxygenation, lung mechanics and alveolar-capillary barriers. Pigs were challenged with LPS (50 μg/kg) intravenously to recapitulate the features of ARDS. When ARDS was well established (T0), animals received hemoadsorption (HA) or sham-hemoadsorption treatment for 3 h. Following another 5-h observation, animals were killed for BALF and lung tissue processing. At baseline, T0, and a series of time points during (2 h) and after HA (or HA-sham) treatment (4, 6 and 8 h), parameters of oxygenation and lung mechanics were recorded. PaO2/FiO2 (a) was measured by using blood samples from femoral artery on a blood gas analysis instrument. The value of mPAP (b) was gained by Swan-Ganz catheter implantation into jugular vein. Resistance (c) and compliance (d) were recorded by using Drager Evita 4 ventilator. EVLWI (e) and PVPI (f) were measured by PiCCO system at indicated time points (baseline, T0, 2, 4, 6 and 8 h following HA or HA-sham treatment). BALF protein (g) was assessed at 8 h after HA (or HA-sham) as described in “Methods”. h The ratio of wet/dry lung weight of animals in both groups was calculated by gravimetric method. i Whole-cell counts in the BALF collected from both groups of pigs were numerated by using a counting plate. j and k were the representative lung histology sections of pigs in LPS + HA (sham) and LPS + HA groups. HE sections are from one representative animal per group. l Lung injury scores were calculated according to ATS report which was in detail described in the “Methods.” Data points represent as mean ± SEM, N = 3–4 of each group and time point. Statistical significance between HA and HA-sham group per point of measurement is shown as *P < 0.05
Table 3
Variables determining oxygenation and lung mechanics in LPS + HA (sham)- and LPS + HA-treated animals
Parameter
Group
Time (h)
Baseline
T0
2 h
4 h
6 h
8 h
PaO2/FiO2 (mmHg)
LPS + HA (sham)
329 ± 55
164 ± 10†
131 ± 20†
129 ± 21†
178 ± 68
169 ± 53
LPS + HA
387 ± 10
183 ± 6†
254 ± 44*
211 ± 31†
264 ± 31
315 ± 22*§
PaCO2 (mmHg)
LPS + HA (sham)
45 ± 4
40 ± 7
45 ± 17
46 ± 14
46 ± 16
42 ± 14
LPS + HA
37 ± 5
53 ± 6†
59 ± 9†
54 ± 3†
51 ± 2
45 ± 3
AaDO2 (mmHg)
LPS + HA (sham)
96 ± 24
170 ± 6
363 ± 129
330 ± 103
371 ± 102†
358 ± 96
LPS + HA
79 ± 10
172 ± 29†
368 ± 68†
368 ± 77†
334 ± 81†
296 ± 66†
PAWPeak (mbar)
LPS + HA (sham)
17.7 ± 1.8
32.0 ± 2.6†
29.7 ± 5.2†
29.7 ± 2.7†
28.3 ± 1.7†
26.7 ± 3.2
LPS + HA
18.9 ± 1.5
29.0 ± 1.0†
26.3 ± 1.9†
26.3 ± 1.8†
24.7 ± 1.8
24.3 ± 2.3
PAWPlateau (mbar)
LPS + HA (sham)
13.3 ± 0.9
21.0 ± 1.0†
22.7 ± 2.9†
23.3 ± 2.4†
21.0 ± 1.0†
21.7 ± 0.9†
LPS + HA
15.3 ± 1.8
24.7 ± 1.3†
22.0 ± 1.2†
21.0 ± 1.0†§
20.3 ± 0.9†§
19.0 ± 0.0*†§
Resistance (mbar/l/s)
LPS + HA (sham)
8.0 ± 1.1
15.0 ± 1.8
17.5 ± 4.6
13.4 ± 3.9
13.7 ± 3.6
13.3 ± 4.0
LPS + HA
8.2 ± 1.0
11.7 ± 1.8
8.8 ± 1.5
8.7 ± 1.2
8.0 ± 1.1
7.2 ± 1.2§
Compliance (ml/mbar)
LPS + HA (sham)
32.6 ± 2.9
20.1 ± 6.1
19.6 ± 7.7
20.2 ± 6.0
20.6 ± 5.0
21.1 ± 5.9
LPS + HA
27.1 ± 2.9
19 ± 2.2†
20.1 ± 1.1
22.5 ± 2.0
22.7 ± 2.8
23.3 ± 2.3
Oxygenation and ventilation parameters in LPS + HA (sham)- and LPS + HA-treated animals at baseline and a series of time points until the end of the experiment (data are mean ± SEM, N = 3–4 of each group; *P < 0.05 when compared between groups; †P < 0.05 when compared with baseline within per group; §P < 0.05 versus T0 within per group). PaO2, oxygen partial pressure; FiO2, inspiratory oxygen fraction; PaCO2, carbon dioxide partial pressure; PAWPeak, peak airway pressure; PAWPlateau, plateau airway pressure
Table 4
Systemic and pulmonary hemodynamic measurements compared between LPS + HA (sham) and LPS + HA groups
Parameter
Group
Time (h)
Baseline
T0
2 h
4 h
6 h
8 h
CO (l/min)
LPS + HA (sham)
6.36 ± 0.41
5.50 ± 1.98
4.86 ± 1.28
5.35 ± 1.13
5.17 ± 1.10
5.56 ± 1.27
LPS + HA
4.98 ± 0.48
4.99 ± 0.78
5.34 ± 0.94
6.08 ± 0.97
5.05 ± 0.89
5.15 ± 0.40
MAP (mmHg)
LPS + HA (sham)
125 ± 6
82 ± 3
92 ± 20
106 ± 21
104 ± 25
96 ± 24
LPS + HA
118 ± 7
85 ± 15
74 ± 9
86 ± 12
82 ± 17
80 ± 16
SVRI (dyn s/cm5/m2)
LPS + HA (sham)
1699 ± 59
1120 ± 154
1813 ± 688
1788 ± 468
1681 ± 354
1454 ± 248
LPS + HA
1992 ± 156
1465 ± 423
1143 ± 231
1210 ± 347
1576 ± 778
1291 ± 461
mPAP (mmHg)
LPS + HA (sham)
23.0 ± 2.6
36.3 ± 5.6
41.3 ± 3.2
38.3 ± 5.8
38.3 ± 5.4
34.0 ± 5.1
LPS + HA
22.7 ± 0.3
37.7 ± 5.2
44.3 ± 5.2
39.3 ± 8.0
35.3 ± 7.8
31.3 ± 10
PVRI (dyn s/cm5/m2)
LPS + HA (sham)
229 ± 31
477 ± 202
518 ± 181
467 ± 85
441 ± 92
343 ± 25
LPS + HA
248 ± 19
404 ± 60
499 ± 72
421 ± 156
483 ± 196
416 ± 145
PAWP (mmHg)
LPS + HA (sham)
9.7 ± 2.3
12.7 ± 3.2
14.7 ± 3.0
12.0 ± 3.1
14.0 ± 4.2
13.0 ± 2.6
LPS + HA
8.3 ± 1.2
11.0 ± 1.2
16.3 ± 1.8
13.0 ± 1.7
11.0 ± 2.0
11.7 ± 3.0
EVLWI (ml/kg)
LPS + HA (sham)
10.1 ± 3.5
13.1 ± 1.4
13.0 ± 0.6
15.9 ± 2.5
13.7 ± 1.0
12.9 ± 2.0
LPS + HA
8.1 ± 0.3
12.4 ± 1.8
12.5 ± 1.5
13.7 ± 1.5
13.0 ± 2.1
10.1 ± 2.3
PVPI
LPS + HA (sham)
3.2 ± 1.0
4.2 ± 0.2
3.7 ± 0.5
4.4 ± 0.5
4.1 ± 0.2
4.0 ± 0.3
LPS + HA
2.5 ± 0.2
4.1 ± 0.5
3.9 ± 1.0
3.6 ± 0.3
3.1 ± 0.7
2.9 ± 0.9
Hemodynamic parameters are shown in the LPS + HA (sham) and LPS + HA groups. Data are mean ± SEM, N = 3–4 of each group; CO, cardiac output; MAP, mean arterial pressure; SVRI, systemic vascular resistance index; MPAP, mean pulmonary arterial pressure; PVRI, pulmonary vascular resistance index; PAWP, pulmonary artery wedge pressure; EVLWI, extravascular lung water index; PVPI, pulmonary vascular permeability index
Hemoadsorption blunts lung edema and histopathological signs of ARDS
Compared with LPS + HA-sham group, HA therapy for ARDS pigs caused a decrease in EVLWI, PVPI, lung wet-to-dry weight ratio and BALF cell count (Fig. 3e, f, h, i; Table 4). However, the changes did not reach statistical difference when compared with LPS + HA-sham group. But HA therapy can significantly reduce total BALF protein as compared to HA-sham treatment (Fig. 3g). These beneficial alterations were further reflected by reduced histologic signs of inflammation and injury (Fig. 3j–l).
Hemoadsorption reduces circulating and alveolar cytokine levels
ELISA assay showed that plasma level of IL-1β and IL-6 induced by endotoxin was significantly blunted by HA treatment compared with HA-sham treatment (Fig. 4a, d). HA also elicited a remarkable decrease in the expression of IL-1β and IL-6 in both BALF and lung homogenate (Fig. 4b, c, e, f). Plasma and lung homogenate levels of IL-8 were also decreased (Fig. 4g, i). BALF levels of TNF-α and IL-17A were significantly reduced by HA treatment (Fig. 4k, n).
Fig. 4
Effect of HA on the production of LPS-induced circulating and pulmonary inflammatory cytokines. Pigs were allocated into LPS + HA (sham) and LPS + HA groups. Plasma was collected at baseline, and at the time point when ALI model was diagnosed (T0) and the end of the experiment schedule (8 h after T0). BALF and lung homogenates were prepared after pigs were euthanized. The systemic and pulmonary cytokine levels of IL-1β (a–c), IL-6 (d–f), IL-8 (g–i), TNF-α (j–l) and IL-17A (m–o) were detected by using ELISA kits. Values are mean ± SEM, N = 4 of each group. *P < 0.05; **P < 0.01; ***P < 0.001 when compared between LPS + HA (sham) and LPS + HA groups; †P < 0.05 versus baseline and §P < 0.05 versus T0 when compared within each group
Hemoadsorption-altered plasma and pulmonary proteome
First, plasma proteome was analyzed. The differentially accumulated proteins (T0 vs baseline) and their dynamic changes after HA/HA-sham treatment (8 h after T0 vs. baseline) are shown in Additional file 5: Fig. S3. These proteins were classified into several categories based on biological process
analysis (Tables 5, 6). We identified four plasma proteins
, i.e., interleukin-1 receptor antagonist protein (IL-1Ra), inter-alpha-trypsin inhibitor heavy chain H4 (ITIH4), matrix metallopeptidase (MMP)-1 and MMP-10, that were up-regulated at T0 in these two groups, but sharply reduced after HA treatment while further increased in HA-sham group (Fig. 5a, b). Differentially expressed proteins (these proteins were comparable at T0 when compared with HA with HA-sham group) after 8-h HA or HA-sham treatment, and their GO annotations are also shown in Additional file 6: Table S2 and Additional file 7: Fig. S4. We then analyzed proteome in BALF and lung homogenate samples. Differentially expressed proteins compared between HA and HA-sham groups are shown in Additional file 8: Table S3, Additional file 9: Table S4, Additional file 10: Table S5, Additional file 11: Table S6. The most five relevant GO categories (P value less than 0.05) are shown in Fig. 5c, d. KEGG pathway analysis showed that these differentially expressed proteins were involved in the canonical signaling pathways (Fig. 5e, f).
Table 5
Ontology groups and associated differentially expressed plasma proteins in the time points of T0 and 8 h after HA-sham treatment versus baseline
aNote that changes are expressed as relative abundance of the plasma proteins at T0 or 8 h after HA-sham treatment compared with baseline within the LPS + HA (sham) group. A fold change ≥ 1.20, p < 0.05 represents more protein abundance in T0 or 8 h versus baseline. By contrast, a fold change ≤ 0.83, p < 0.05 represents less protein abundance in T0 or 8 h versus baseline
Table 6
Ontology groups and associated differentially expressed plasma proteins in the time points of T0 and 8 h after HA treatment versus baseline
GO biological process
Accession
Protein name
Fold change over baselinea
T0/baseline
8 h/baseline
Acute-phase response/acute inflammatory response
Q29014
Alpha-1 acid glycoprotein (Fragment)
2.70
0.87
K9J6H8
Alpha-2-macroglobulin
1.82
1.01
I3L6K3
C-reactive protein
1.43
2.50
F1RJ76
C-reactive protein
1.27
1.32
Q8SPS7
Haptoglobin
2.08
1.00
P79263
Inter-alpha-trypsin inhibitor heavy chain H4
1.89
1.78
F1SH92
Inter-alpha-trypsin inhibitor heavy chain H4
1.47
1.19
Q29056
Interleukin-1 receptor antagonist protein
2.44
1.44
F1S9B8
Serum amyloid A protein
1.64
1.35
Regulation of immune system process
P01025
Complement C3
1.50
1.34
F1SMJ1
Complement component C7 (Fragment)
1.23
1.07
A5PF00
B-factor, properdin
2.50
0.95
F1RMN7
Hemopexin
1.85
1.08
L8B0S2
IgG heavy chain
1.82
1.00
L8B0W9
IgG heavy chain
1.30
0.94
K7ZPU8
IgG heavy chain constant region (Fragment)
1.59
0.72
Q4Z8N7
Plasma platelet-activating factor acetylhydrolase
1.20
1.38
P28491
Calreticulin
0.81
1.29
B0LUW3
Chemerin
0.62
0.79
F1STZ4
Complement C1q subcomponent subunit A
0.83
0.82
Q29041
Ficolin-2
0.77
0.72
A5A758
Keratin 1 (Fragment)
0.53
0.69
C4PGL9
Mannan-binding lectin serine peptidase 2
0.65
0.75
Defense response/response to stress
A2SW51
Monocyte differentiation antigen CD14
1.64
1.60
P52552
Peroxiredoxin-2 (Fragment)
1.59
1.64
P32195
Protegrin-2
1.25
1.05
B3STX9
Prothrombin
1.28
1.01
F5XVC2
von Willebrand factor
1.35
1.07
Q6QR67
Resistin
1.79
1.52
Proteolysis
Q9GMA6
Alpha-1-antichymotrypsin 2
1.47
1.03
F1SCF0
Alpha-1-antitrypsin
2.04
0.87
C9VZX4
Matrix metallopeptidase 1
1.47
1.22
C9VZX5
Matrix metallopeptidase 10
1.43
1.21
Coagulation
P14460
Fibrinogen alpha chain (Fragment)
1.54
3.30
P14477
Fibrinogen beta chain (Fragment)
1.43
1.78
F1RQ75
Coagulation factor IX
0.78
0.60
F1RPW2
Coagulation factor V
0.79
0.67
Q19AZ7
Coagulation factor VII isoform b protein
0.72
0.81
K7GQL2
Coagulation factor XIII, A1 polypeptide
0.51
0.54
Negative regulation of blood coagulation
I3LRJ4
Vitamin K-dependent protein C
0.74
0.64
Metabolic process
F1S1G8
Amine oxidase
1.64
1.01
P01965
Hemoglobin subunit alpha
2.17
1.11
F1RII7
Hemoglobin subunit beta
1.89
1.22
Q29052
Inter-alpha-trypsin inhibitor heavy chain H1
1.32
1.08
F8SIP2
EGF-containing fibulin-like extracellular matrix protein 1
0.80
1.09
O02668
Inter-alpha-trypsin inhibitor heavy chain H2
0.74
0.64
I3LL80
L-lactate dehydrogenase
0.81
0.65
Q29126
Protein WAP-3
0.31
0.84
Regulation of lipid storage
A0A0F6TNY5
APOB O
1.43
1.09
Q29433
Apolipoprotein B (Fragment)
2.17
1.21
Q2LE37
Apolipoprotein M
1.23
1.04
O97674
Lipoprotein lipase (Fragment)
0.62
0.64
D3Y264
Apolipoprotein C-II
0.80
0.63
F1RM45
Apolipoprotein E
0.75
0.89
Q03472
Apolipoprotein R
0.72
0.60
Q8WMN7
Plasma phospholipid transfer protein
0.79
0.85
Cellular metal ion homeostasis
I3VKE6
Ceruloplasmin
1.30
1.07
Q6YT39
Lactotransferrin
1.61
1.33
P09571
Serotransferrin
2.33
0.91
D7RK08
Transferrin receptor protein
1.45
1.30
Transport
F1RUN2
Serum albumin
2.08
1.01
P50390
Transthyretin
1.33
0.89
Positive regulation of cell differentiation
Q0PM28
Pigment epithelium-derived factor
1.32
1.11
Multicellular organismal process
Q711S8
Secreted phosphoprotein 24
0.74
0.72
O11780
Transforming growth factor-beta-induced protein ig-h3
0.83
0.97
P67937
Tropomyosin alpha-4 chain
0.81
1.23
P00761
Trypsin
0.82
0.85
aNote that changes are expressed as relative abundance of the plasma proteins at T0 or 8 h after HA treatment compared with baseline within the LPS + HA group. A fold change ≥1.20, P < 0.05 represents more protein abundance in T0 or 8 h versus baseline. By contrast, a fold change ≤0.83, P < 0.05 represents less protein abundance in T0 or 8 h versus baseline
Fig. 5
Differentially expressed plasma, BALF and lung proteins identified with iTRAQ in LPS + HA (sham)- versus LPS + HA-treated pigs. a and b four plasma proteins that were most differentially expressed after 8-h treatment in LPS + HA (sham)- versus LPS + HA-treated pigs. Note that after LPS infusion, these proteins were up-regulated (T0/baseline); however, after HA treatment, their expression were decreased. By contrast, they were further increased after HA-sham treatment. Functional annotation for differentially expressed BALF (c) and lung homogenate (d) proteins by HA and HA-sham treatment are shown. Red bars represent the numbers of differentially expressed proteins based on three main categories: cellular component, biological process and molecular function. Enriched KEGG pathway analysis for differentially expressed BALF (e) and lung homogenate (f) proteins by HA and HA-sham treatment are shown. Red bars represent the numbers of proteins in a given pathway that differentially expressed between groups
Discussion
In this current study, we tested the efficacy of “sorbent strategy”-based HA on a porcine ARDS model and found that HA reduced circulating and alveolar levels of proinflammatory cytokines, improved oxygenation and attenuated lung injuries in the exudative phase. This provides some clue that HA330 cartridge may be a novel potential weapon fighting against the “cytokine storm” on the alveolar-capillary membrane barrier.
The most commonly used large-animal models of ARDS include endotoxin infusion, repeated lavage, oleic acid and smoke/burn injury [17]. To reproduce the most known risk factor and etiology for ARDS, which is sepsis [18], we systemically administrated endotoxin (LPS) to mimic the clinically relevant sepsis-induced ARDS. The susceptibility to LPS is highly variable and differs among different animals. Pigs, sheep, calves, and cats are more sensitive to LPS challenge. Low dosage of LPS (μg/kg range) can induce significant ARDS-like features in these animals. In contrast, animals such as rodents or dogs require much higher doses to develop lung injury (mg/kg range). This different vulnerability to LPS may be induced by the pulmonary intravascular macrophages (PIM), a lung resident population of mature macrophage [19]. 8–100 μg/kg of LPS has been used in several previous studies to develop porcine ARDS model [12, 20, 21]. In our study, low amount of LPS (50ug/kg in 500 ml saline for 2 h) can also induce the pigs to develop an abrupt decrease in oxygenation and arterial pressure and a decrease in systemic vascular resistance, needing rapid fluid resuscitation (10–20 ml/kg/h of saline) and the usage of vasopressor infusion (0.5–1.5 μg/kg/min of norepinephrine).
In most recent large-animal studies, the diagnosis of experimental ARDS is ambiguous without definite criteria [12, 18, 21, 22]. To determine whether ARDS really occurred, we adopt the four diagnostic criteria released by ATS official statement on the definition of ARDS in animals [14]. ARDS model was initially diagnosed when PaO2/FiO2 is less than 200 mmHg with a PEEP at 5 cmH2O (criteria (a) moderate ARDS in human beings according to Berlin definition). Then, the ARDS model was further assessed with other criteria listed as follows: (b) permeability. Permeability assessment was performed by using four parameters, i.e., EVLWI, PVPI, BALF protein and the ratio of wet to dry lung weight (W/D ratio). EVLW is the amount of interstitial and alveolar fluid [23]. Previous studies showed that EVLW indexed to body weight (EVLWI) is well correlated with the value obtained by gravimetry and can independently predict mortality in septic and ARDS patients [19]. We found that both EVLWI and W/D ratio were significantly increased after LPS infusion, indicating an exudative edema phase (Fig. 1; Table 2). The permeability of lung epithelium barrier can also be calculated by PVPI [24]. PVPI in this model was increased to 5.6 ± 0.5 at T0 when ARDS was diagnosed (Fig. 1; Table 2), indicating high permeable (rather than hydrostatic) pulmonary edema because it was reported that a PVPI value of 3 can distinguish these two forms of pulmonary edema [24]. Accordingly, BALF protein concentration, another leakage marker [14], was also increased after LPS infusion (Fig. 1g). (c) Histology. To our knowledge, this is the first large-animal study to assess histologic changes at the time point that ARDS was initially diagnosed by oxygenation and ahead of therapy implementation. The major histologic findings are shown in Fig. 1j–l. It is noteworthy that LPS i.v. infusion causes only modest lung edema (perivascular edema, Additional file 4: Fig. S2) as compared to ARDS patients, because the endothelium barrier is more resistant to the damage induced by LPS [19]. (d) Inflammation. We found that both circulating and alveolar inflammatory cytokines were elevated, indicating an acute “cytokine storm” was elicited in systemic and lung milieu by i.v. infusion of LPS.
Thereafter, we conducted subsequent studies to explore the “therapeutic,” rather than “prophylactic” effect of hemoadsorption (HA) on the well-established (or far-developed, rather than “immature”) ARDS model. HA was performed with the HA330 neutral microporous resin cartridge specially designed for the absorption of medium-sized inflammatory cytokines. First, we found that HA treatment increased PaO2/FiO2 gradually (Fig. 3). Several previous studies in septic patients attributed this beneficial effect to the improved hemodynamics [10, 25]. However, a previous experimental study showed that zero-balanced high-volume continuous veno-venous hemofiltration (CVVH) could improve arterial oxygenation without systemic or pulmonary hemodynamics improvement [9]. We also found that animals treated with or without HA330-based hemadsorption did not differ in their levels of MAP, SVRI, MPAP and PVRI (Table 4). Considering that HA therapy elicited a trend in reducing lung water and the permeability of alveolar-capillary membrane barrier (Fig. 3e–i), we assume that oxygenation improvement should be partly due to the reduction of alveolar fluid leakage after clearing the peak concentration of alveolar cytokines, corresponding with the “peak concentration hypothesis” for EBP modality [26]. Lung local cytokines removal may be the result of passive spillover or active transport [26]. Notably, a recent clinical study showed that the circulating and BALF levels of IL-17A were significantly increased in ARDS patients and predicted an increased influx of alveolar neutrophils, alveolar permeability and organ dysfunction [27]. Thus, reduced BALF level of IL-17A in HA treatment group may be one of the reasons for fewer lung inflammatory cells and decreased acute lung injury. Taken together, by direct/indirect removal of a variety of pathogenic proinflammatory mediators that over-expressed in plasma and lung, HA timely blunted the “cytokine storm” in the process of ARDS and restored immunologic balance at a much lower set-point. These findings were in line with a recent small clinical study on septic-induced ARDS patients [28].
In the last step, we also examined whether HA can effect the whole proteomes in plasma and lung, which has not been previously reported. We found four plasma proteins that were most differentially regulated by HA and HA-sham therapy, i.e., IL-1Ra, MMP-1, MMP-10 and ITIH4 (Fig. 5a, b). Soluble IL-1Ra, an important member in IL-1 family of cytokines [29], was dramatically elevated in ARDS and septic patients [30, 31]. A persistent elevated level of IL-1Ra indicates immunoparalysis, which greatly contributes to the later deaths who survive the initial cytokine storm in ARDS [32]. ITIH4 is a plasma glycoprotein that belongs to a serine protease inhibitor family and acts as an acute-phase protein in several diseases [33]. However, there is a lack of studies aiming to determine the role of ITIH4 as a potential diagnostic or prognostic indicator for ARDS. The matrix metalloproteinases (MMPs) are a family of proteolytic enzymes with the capacity of degrading the extracellular matrix component, thus causing tissue damage in the pathological process [34]. Previous studies were largely focused on the BAL fluid level of MMPs (including MMP2, MMP8 and MMP9) and found an elevated expression pattern [35]. However, the circulating and BALF levels of MMP-1 (interstitial collagenase) and MMP-10 (Stromeolysin 2) in ARDS animals or patients are remained largely unknown. Collectively, we concluded a composite of plasma biomarkers with IL-1Ra, MMPs and ITIH4 may be useful to predict the severity of ARDS. Of course, this hypothesis needs further verification.
We also determined the role of HA330 cartridge-based HA on BALF and lung homogenate proteome (Additional file 8: Table S3, Additional file 9: Table S4, Additional file 10: Table S5, Additional file 11: Table S6). Notably, we found that the BALF level of secreted histone H2A, H2B and H4 was significantly blunted after HA therapy compared with HA-sham-treated pigs. Extracellular histones are the constituent of neutrophil extracellular traps (NETs) structures that ensnare and kill bacteria [36]. Elevated extracellular histones in BALF samples from humans with ARDS have been reported [37]. Also, instillation of neutralizing anti-histone H2A/H4 antibody reduced experimental ARDS severity [38]. Because extracellular histones origin from actively secretion by activated inflammatory cells, or from passively release by necrotic cells, we concluded that HA can significantly reduced the BALF level of histones by attenuating inflammatory lung injuries. BALF and lung level of Surfactant protein (SP)-B and SP-C were also significantly up-regulated by HA versus HA-sham treatment. Previous studies showed decreased levels of SP-A, SP-B and SP-C in BALF of ARDS patients [39]. Thus, HA treatment may improve oxygenation by restoring the alveolar levels of surfactant proteins. Collectively, we showed with the first experience that HA330-directed HA performance has a profound impact on plasma and lung proteome in a sepsis-induced ARDS porcine model.
Our studies have some strength. First, we comprehensively assessed the lung histologic features and other biomarkers when the ARDS model was initially diagnosed by oxygenation. Second, we first assessed the effect of HA on experimental ARDS model by using iTRAQ-labeled proteomic technology. However, our studies also have some limitations. This is a small sample animal study. Also, the effect of HA330 directed HA should be further tested by other ARDS models. Third, the experimental data cannot be directly introduced into the real clinical practice. There is still a long way to go that HA-330 cartridge-based HA can be used in ARDS patients.
Conclusions
In conclusion, HA330 resin-based HA attenuated experimental ARDS by blunting circulating and lung “cytokine storm,” improving permeability of alveolar barrier and promoting the recovery of the disordered proteomes.
XX designed, made, analyzed the experiments and drafted the manuscript. CJ designed and made the experiments. L Sa participated in the design and performance of the experiments. F Xiao, Y Li and H Dai participated in the analysis of the data and the critical revision of the article. C Wang contributed to the conception and design of the study, the analysis and interpretation of the data, revision of the article and final approval of the version to be published. All authors read and approved the final manuscript.
Acknowledgements
We would like to thank Dr. Mingxu Shang, Dr. Hangyong He, Dr. Xiao Tang and Dr. Bing Sun, Department of Respiratory and Critical Care Medicine, Beijing Chao-Yang Hospital for their for their excellent technical assistance.
Competing interests
The authors declare that they have no competing interests.
Availability of supporting data
All the data are available and will be submitted if required.
Consent for publication
All the coauthors approve the publication of this manuscript.
Ethical approval and consent to participate
This study was approved by the Institutional Animal Experiment Committee of Beijing Hospital.
Funding
This work was supported by Grants from National Natural Science Foundation of China (Nos. 81490534, 81490530, 81430001).
Publisher’s Note
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Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made.
Authors’ Affiliations
(1)
National Clinical Research Centre for Respiratory Diseases, Beijing Hospital
(2)
Department of Surgical Intensive Care Medicine, Beijing An Zhen Hospital, Capital Medical University
(3)
Department of Pulmonary and Critical Care Medicine, China-Japan Friendship Hospital
(4)
Department of Pulmonary and Critical Care Medicine, Beijing Hospital
(5)
Key Laboratory of Geriatrics, Beijing Hospital and Beijing Institute of Geriatrics, Ministry of Health
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