Hypothermic properties of dexmedetomidine provide neuroprotection in rats following cerebral ischemia‑reperfusion injury

Introduction

Mortality and morbidity rates as a result of cardiac arrest (CA) remain high despite steady advances in therapeutic approaches over the past decades (1). Post-resuscitation neurological dysfunction is a major cause of mortality in patients following successful cardiopulmonary resuscitation (CPR) (2,3). Therefore, it is vital to research strategies to protect neurological function in patients following CA.

Although CA can lead to ischemia/reperfusion (I/R) injury in every organ in the body, it is especially detrimental to the brain and the heart. The principal pathological cause of organ damage is excessive apoptosis and autophagy (4,5), the extent of which has been found to correlate with poor neurological prognosis (6–8). A number of studies have demonstrated that hypothermia can attenuate neurological damage following I/R injury by reducing neural apoptosis and preventing autophagy overactivation (4,9,10). Therefore, it has been recommended as a potential treatment in patients who were successfully resuscitated following CA (11).

Apoptosis is a form of cell death that is mediated by several proteins, including Bax, Bcl-2, 70 kDa heat shock protein (HSP70) and cysteinyl aspartate specific proteinase (Caspase-3) (12,13). Bax and Bcl-2 are members of the Bcl-2 family of molecular protein factors that can reflect the extent of cellular apoptosis (14); whereas HSP70 is a highly conserved molecular chaperone that serves an important role in cellular adaptation to stress, a requisite for cell survival (15). Lastly, Caspase-3 is a commonly probed apoptosis marker, as it takes part in the execution-phase of the apoptotic pathway (13,16,17).

Autophagy is the primary mechanism by which cytosolic proteins and organelles are degraded (18). However, excessive autophagy activation in neurocytes damaged by I/R can lead to non-apoptotic cell death (19,20), which is called autoghagic programmed cell death. Beclin1 activates critical steps in autophagy, including the formation and maturation of autophagosomes (21,22). In addition, Bax and Bcl-2 have also been demonstrated to regulate autophagy (12). In fact, it has been well documented that the crosstalk between autophagy and apoptosis pathways is mediated at least in part by the functional and structural interaction between Beclin1 and Bcl-2 (23).

Dexmedetomidine (Dex) is a highly selective α2-adrenergic receptor agonist that is commonly used as a sedative and analgesic in the intensive care unit (24); it has been reported to display synergistic effects with hypothermia (25,26). Consequently, based on previous observations that hypothermia can alleviate neuronal damage following CA, it was hypothesized in the present study that Dex administration after CA may result in improved neural function and reduced apoptosis and autophagy. The present study also aimed to investigate the possible mechanism by which Dex improves cognitive function.

Materials and methods

Animal preparation and Experimental protocol

All operations and euthanasia were performed under anesthesia induced by an intraperitoneal (i.p.) injection of 3.6% chloral hydrate solution (3.6 g chloral hydrate crystal diluted with 100 ml distilled water) at a concentration of 360 mg/kg, and the best efforts were made to minimize animal suffering.

A total of 72, male Sprague-Dawley rats [age, 17 and 18 weeks; weight, 430±45 g; JOINN Laboratories (China) Co., Ltd.] were recruited successfully. They were provided food and water ad libitum, and housed at 25°C, with freshly ventilator delivered atmosphere and a 12 h light/dark cycle. The procedure of animal CA and CPR were performed as described previously (4). Endotracheal intubation was performed prior to left/right femoral arteriovenous catheterization. Animals were ventilated with a volume-controlled ventilator (Institute of Cardiopulmonary Cerebral Resuscitation, Guangdong, China), with a tidal volume of 6 ml/kg, a fraction of inspired oxygen (FiO2) of 0.21, and a ventilation rate of 100 breaths per min. Continuous arterial blood pressure was monitored via an intra-arterial pressure sensor suite (Philips Medical Systems, Inc.) and an electrocardiogram (Anhui Zhenghua Biological Instrument Equipment Co., Ltd.). Baseline arterial blood gas analysis was performed 10 min after the surgical procedure. An equal volume (0.5 ml) of normal saline was supplemented into the venous catheter immediately after arterial blood collection. CA was induced in the animals by reducing mechanical ventilation and occluding the tracheal catheter. For CPR, external chest compression (250 bpm) and mechanical ventilation (6 ml/kg and 100 bpm) was performed after a period of 5 min under systolic blood pressure <25 mmHg. After 10 sec of CPR all rats were administered a bolus injection of epinephrine (10 µg/kg, diluted to 0.5 ml) in the right femoral vein. In addition to epinephrine, before CPR execution, one group of rats received an i.p. injection of Dex (50 µg/kg (27), diluted to 0.5 ml; D group) whereas another group received an i.p. injection of 0.9% normal saline (0.5 ml; N group). ROSC achievement was defined as the presence of an autonomic cardiac rhythm and a mean arterial blood pressure >60 mmHg. At this point, chest compressions were stopped, a FiO2 of 100% was maintained for 15 min after ROSC, decreased to 45% for a further 15 min and then decreased to 21% until the animal exhibited spontaneous respirations. Resuscitation procedures were terminated if animals were unresponsive to CPR for 10 min. After 2 h of monitoring animal vital signs, rats returned to consciousness, were placed into a thermostabilized (25°C) cage for rehabilitation and euthanized either 12 (N-12, n=15; D-12, n=15) or 24 h (N-24, n=14; D-24, n=13) later. A total of 9 rats died during the recovery period in the cage due to airway edema and sputum obstruction, which was certified following autopsy. Rats belonging to the blank control group (BC; n=6) received identical surgical and anesthetic treatments as the experimental rats with the exception of CA and CPR.

Critical parameters, including core (rectal) temperature and blood pressure were monitored continuously for 120 min (timed from the first sign of ROSC) after CPR until the rats regained consciousness. Within the same timeframe, arterial blood gas was also analyzed 30 and 120 min after CPR.

Neurological deficit scores (NDS)

NDS is a common procedure for evaluating neurological dysfunction by using a hierarchical scoring system based on respiratory pattern, consciousness, sensory and motor function and behavioral responses (4). Every animal was evaluated 12 or 24 h following return of spontaneous circulation (ROSC). The NDS items were collected by investigators that have been specially trained, who were blinded to the experimental groups. Individual scores were subsequently combined to produce the final NDS score. A score of 80 is considered normal whereas a score of zero is considered brain dead (28).

Collection of rat hippocampal tissues

After the NDS scores were obtained, rats were anesthetized using a combination of an i.p. injection of 3.6% chloral hydrate solution at 360 mg/kg and an intracardial injection of 500 mg/kg 10% potassium chloride solution. The hippocampus was rapidly removed from the cerebrum of the rat. The left half was snap frozen using liquid nitrogen before storage at −80°C to be used later for western blot analysis of Bcl-2, Bax, HSP70 and Beclin1 protein expression. The right half of the hippocampus was fixed in 4% paraformaldehyde for 24 h at 4°C and subsequently embedded in paraffin for analysis using histology techniques.

Western blot analysis of Bcl-2, Bax, HSP70 and Beclin1 expression in the rat hippocampus

Hippocampal tissue protein was extracted with 400 µl RIPA and 4 µl PMSF (Beyotime Institute of Biotechnology). Samples were then homogenized on the ice and centrifuged in a refrigerated centrifuge (12,000 × g for 10 min at 4°C). Protein concentration in the supernatant from hippocampal homogenate was determined using a Bicinchoninic Acid Assay kit (Beyotime Institute of Biotechnology). A total of 50 µg of protein obtained from the hippocampus were separated by 10 or 12% SDS-PAGE before transferal to a PVDF membrane. Each membrane was blocked in 5% non-fat milk diluted in TBS supplemented with 0.1% Tween-20 (TBST) for 1 h at 4°C. The membranes were then incubated overnight at 4°C with primary antibodies against Bcl-2 (1:1,000; cat. no. ab196495), Bax (1:1,000; cat. no. ab32503), HSP70 (1:1,000; cat. no. ab137680), Beclin1 (1:1,000; cat. no. ab62557) or Glyceraldehyde-3-phosphate dehydrogenase (GAPDH; 1:800; cat. no. ab9485); all primary antibodies applied for western blot analysis were purchased from Abcam. The following day, the membranes were rinsed with TBS-T and subsequently incubated with a biotin-conjugated goat anti-rabbit IgG secondary antibody (1:5,000; cat. no. ab222773; Abcam) at room temperature for 1 h. Protein bands were visualized using an ECL reagent (Biological Industries Israel Beit Haemek Ltd.). Densitometric analysis was performed using Quantity One 1-D analysis software (version 4.6.9; Bio-Rad Laboratories, Inc.); the protein levels of Bcl-2, Bax, HSP70 and Beclin1 were all normalized to GAPDH.

Immunohistochemistry analysis of Caspase-3

Paraffin-embedded hippocampal tissue was cut into 5 µm sections using a sledge microtome. The tissue was deparaffinized using xylene and rehydrated in a series of descending concentrations of ethanol. Antigen retrieval was completed by boiling in citric acid buffer (10 mM, pH 6.0) at 95°C for 15 min. 0.5% Triton X-100 (Beyotime Institute of Biotechnology) was used for membrane permeabilization. The slides were blocked at 37°C for 2 h in 5% bovine serum albumin (BSA; Beyotime Institute of Biotechnology) diluted in TBS and subsequently incubated in anti-caspase-3 antibody (1:100; cat. no. ab4051; Abcam) diluted in TBS supplemented with 5% BSA overnight at 4°C. The following day, the sections were rinsed in TBS prior to incubation with a biotin-conjugated goat anti-rabbit secondary antibody (1:500; cat. no. ab222773) for 1 h at 37°C. The secondary antibody was washed off using TBS and the slides were incubated under 37°C for 5–10 min in a solution containing 0.02% diaminobenzidine (DAB) and 0.01% H2O2 and then counterstained using hematoxylin and eosin (H&E) at 37°C for 10 min. The slides were imaged using a light microscope (Olympus BX53; Olympus Corporation). Cells exhibiting brown staining were considered Caspase-3 positive and were counted using the Leica software analysis system (Q550CW; Leica Microsystems, Inc). Each group was observed in four different fields of view; 100 cells were observed in the field of vision and then caspase-3 positive cells were calculated. Counting was performed by a specialized pathologist who was blind to the experimental groups.

Transmission electron microscopy (TEM)

The paraffin-embedded tissues were also used for histological analysis using TEM. This tissue was sliced using a microtome into ultra-thin sections (~40–50 nm). The sections were then stained with 2.0% (w/v) lead citrate at 4°C for 10 min and evaluated using a Hitachi H-600 transmission electron microscope (Hitachi, Ltd.) in a blinded fashion. For every section, four different TEM micrographs each representing independent fields of view were analyzed.

Statistical analysis

All experimental data are presented as the mean ± SD. A t-test was used to compare the means between the two groups. Multiple-comparison analyses performed in this study were confirmed using Levene's test for the equality of variances. A one-way ANOVA was applied to assess holistic differences between groups for each variable, and Bonferroni post-hoc test was used for multiple comparisons. The software package used to perform the analysis was IBM SPSS Statistics 22.0 (IBM Corp.). P<0.05 was considered to indicate a statistically significant difference.

Results

Animal hemodynamic, physiological, and resuscitation data

The experimental scheme of animal treatment for the present study is detailed in Fig. 1. No statistically significant differences were observed in operation, hemodynamic stabilization, asphyxia, CA and CPR time between the resuscitation groups (Table I). In addition, no significant differences were identified between the groups with regards to the respiration rate, mean aortic blood pressure, arterial blood pH, oxygen and carbon dioxide partial pressure, oxygen saturation and lactic acid during baseline, at either 30 min or 2 h after ROSC (Table II). Core body temperatures and heart rates in the D group decreased over time, and began to exhibit statistically significant reductions compared with the N group from 40 and 80 min post-ROSC, respectively, up to post-ROSC 120 min when the analyses ended (both P<0.05; Figs. 2 and 3; Table II).

Figure 1. Experimental scheme for animal treatment. SBP, systolic blood pressure; BGA, blood gas analysis; NDS, neurological deficit scores; CA, cardiac arrest; CPR, cardiopulmonary resuscitation; ROSC, return of spontaneous circulation.

Figure 2. Measurement of rat core (rectal) temperature from baseline up to 120 min post-ROSC. The core temperatures between the two groups exhibited statistically significant differences from 40 min onwards after ROSC (black box). *P<0.05 vs. N group. D group, dexmedetomidine treatment group; N group, normal saline group; PR, post-ROSC.

Figure 3. Heart rate measurements in rats from baseline to 120 min post-ROSC. The heart rates between the two groups exhibited statistically significant differences from 80 min after ROSC (black box). *P<0.05 vs. N group. bpm, beat per minute; D group, dexmedetomidine group; N group, normal saline group; PR, post-ROSC; ROSC, return of spontaneous circulation.

Table I. Cardiac arrest time and associated resuscitation data.

Table I.

Cardiac arrest time and associated resuscitation data.

Group	Valid rats (n)	Time of operation (sec)	Time of stabilization for baseline (sec)	Time from asphyxia to SBP <25 mmHg (sec)	Time of SBP <25 mmHg (sec)	Time from resuscitation to ROSC (sec)
N	29	485.61±62.47	589.24±15.72	221.26±36.43	272.34±36.75	86.41±32.67
D	28	505.73±58.32	596.12±12.67	234.82±32.48	268.28±38.74	89.64±29.53

[i] D, dexmedetomidine group; N, normal saline group; ROSC, return of spontaneous circulation; SBP, systolic blood pressure.

Table II. Animal physiological data and arterial blood gas analysis.

Table II.

Animal physiological data and arterial blood gas analysis.

A, N (n=29)
Timepoint	Tc (°C)	HR (bpm)	RR (bpm)	MAP (mmHg)	pH	PaO2 (mmHg)	PaCO2 (mmHg)	SO2c (%)	Lac (mg/dl)
Baseline	37.25±0.48	262.84±39.42	79.87±2.81	92.35±25.52	7.37±0.07	95.43±18.71	40.35±5.41	95.24±6.45	1.2±1.17
PR-0.5 h	36.09±0.47	241.24±47.41	78.96±0.68	65.38±12.84	7.21±0.13	73.54±21.75	55.83±17.68	90.40±9.82	7.1±2.43
PR-2 h	36.85±0.53	251.47±51.84	92.42±13.24	89.49±26.75	7.28±0.09	86.68±24.24	47.37±8.54	92.86±8.23	3.6±1.76
B, D (n=28)
Timepoint	Tc (°C)	HR (bpm)	RR (bpm)	MAP (mmHg)	pH	PaO2 (mmHg)	PaCO2 (mmHg)	SO2c (%)	Lac (mg/dl)
Baseline	37.13±0.39	258.46±42.43	77.65±2.51	99.50±21.38	7.38±0.03	97.64±15.61	41.86±6.23	96.13±3.46	1.5±0.99
PR-0.5 h	35.75±0.41	229.28±42.37	79.86±0.67	61.12±13.58	7.25±0.12	71.46±19.73	52.16±13.26	91.53±7.43	7.2±1.92
PR-2 h	34.12±0.35a	212.48±36.53a	88.76±11.47	85.83±21.44	7.30±0.08	88.47±18.31	44.49±7.64	93.43±9.37	3.2±1.18

a P<0.05 vs. N group. N, normal saline group; D, dexmedetomidine group; HR, heart rate; Lac, lactic acid; MAP, mean aortic pressure; PaCO₂, partial pressure of carbon dioxide; PaO₂, partial pressure of oxygen; PR, post-ROSC; bpm, beats per minute; RR, respiratory rate; SO_2c, oxygen saturation; T_c, core temperature (rectal).

Neurological outcome

NDS was determined before the rats were euthanized at 12 or 24 h post-ROSC. The mean NDS value of rats in the N-12 (43.5±5.7) and N-24 (50.6±5.1) groups was significantly lower compared with the BC group (80.0±0.0; P<0.05; Fig. 4). However, post-ROSC NDS was higher in the D-12 (56.2±6.1) and D-24 (63.4±4.9) groups compared with their respective N-12 and N-24 timepoints (P<0.05; Fig. 4). These findings suggested that the use of Dex post-ROSC in rats improved neurological outcomes after CA compared with untreated animals.

Figure 4. Rat neurological deficit scores. NDSs were evaluated 12 and 24 h after ROSC in the presence of normal saline or dexmedetomidine. *P<0.05. ROSC, return of spontaneous circulation; BC, blank control group; D-12, dexmedetomidine group 12 h post-ROSC; D-24, dexmedetomidine group 24 h post-ROSC; N-12, normal saline group 12 h post-ROSC; N-24, normal saline group 24 h post-ROSC.

Intracellular Bax, Bcl-2, HSP70 and Beclin1 protein expression levels in the hippocampus

Bax expression was found to be greater in the N-12 (0.024±0.002) and N-24 (0.022±0.006) groups post-ROSC compared with the BC group (0.003±0.000) (P<0.05; Fig. 5A). In addition, Bax expression was significantly lower in the D-12 (0.017±0.001) and D-24 (0.006±0.004) groups post-ROSC compared with the respective N-12 and N-24 timepoints (P<0.05; Fig. 5A). Bcl-2 expression was significantly reduced in the N-12 (0.019±0.001) and N-24 (0.014±0.001) groups post-ROSC compared with the BC group (0.022±0.000) (P<0.05; Fig. 5B). However, Bcl-2 expression was significantly higher in the D-12 (0.025±0.001) and D-24 (0.024±0.006) groups post-ROSC compared with their respective N-12 and N-24 timepoints (P<0.05; Fig. 5B). HSP70 expression was higher in the N-12 (0.45±0.07) and N-24 (0.41±0.05) groups post-ROSC compared with the BC group (0.32±0.00) (P<0.05; Fig. 5C). In addition, HSP70 expression was higher in the D-12 (0.56±0.10) and D-24 (0.54±0.06) groups compared with the respective N-12 and N-24 timepoints (P<0.05; Fig. 5C). Beclin1 expression was higher in the N-12 (0.43±0.05) and N-24 (0.39±0.04) groups post-ROSC compared with the BC group (0.15±0.00) (P<0.05; Fig. 5D). However, Beclin1 expression was lower in the D-12 (0.31±0.06) and D-24 (0.25±0.03) groups post-ROSC compared with their respective N-12 and N-24 timepoints (P<0.05; Fig. 5D).

Figure 5. Western blotting results. All data values were normalized to the values of BC group (as level ‘1’). (A) Measurement of Bax protein. The expression levels were in the rat hippocampus from each treatment group 12 and 24 h after ROSC, in the presence of normal saline or dexmedetomidine. *P<0.05. BC, blank control group; D-12, dexmedetomidine group 12 h post-ROSC; D-24, dexmedetomidine group 24 h post-ROSC; N-12, normal saline group 12 h post-ROSC; N-24, normal saline group 24 h post-ROSC; ROSC, return of spontaneous circulation. (B) Measurement of Bcl-2 protein. The expression levels were in the rat hippocampus from each treatment group 12 and 24 h after ROSC, in the presence of normal saline or dexmedetomidine. *P<0.05. BC, blank control group; D-12, dexmedetomidine group 12 h post-ROSC; D-24, dexmedetomidine group 24 h post-ROSC; N-12, normal saline group 12 h post-ROSC; N-24, normal saline group 24 h post-ROSC; ROSC, return of spontaneous circulation. (C) Measurement of HSP70 protein. The expression levels were in the rat hippocampus from each treatment group 12 and 24 h after ROSC, in the presence of normal saline or dexmedetomidine. *P<0.05. BC, blank control group; D-12, dexmedetomidine group 12 h post-ROSC; D-24, dexmedetomidine group 24 h post-ROSC; HSP70, heat shock protein 70 kDa; N-12, normal saline group post-ROSC 12 h; N-24, normal saline group 24 h post-ROSC; ROSC, return of spontaneous circulation. (D) Measurement of Beclin1 protein. The expression levels were in the rat hippocampus from each treatment group 12 and 24 h after ROSC, in the presence of normal saline or dexmedetomidine. *P<0.05. BC, blank control group; D-12, dexmedetomidine group 12 h post-ROSC; D-24, dexmedetomidine group 24 h post-ROSC; N-12, normal saline group 12 h post-ROSC; N-24, normal saline group 24 h post-ROSC; ROSC, return of spontaneous circulation.

Measurement of apoptosis in the rat hippocampus

Neuronal apoptosis was determined by counting the number of Caspase-3-positive staining cells located in the CA1 region of the hippocampus. The intense staining of surrounding tissues was impacted by the time of DBA coloration and the brown staining inside cells was defined as apoptosis-positive. The number of apoptotic neurons were demonstrated to be more abundant in the N-24 group compared with the BC group (P<0.05; Fig. 6). However, fewer hippocampal neurons were stained positive for Caspase-3 in the D-24 group compared with N-24 group (P<0.05; Fig. 6).

Figure 6. Comparison of Caspase-3 positive cells by immunohistochemical analysis. IHC techniques were used in the rat CA1 region of the hippocampus 24 h after ROSC, in the presence of normal saline or dexmedetomidine. (A-C) Brown globules indicate Caspase-3-positive expression, which is indicative of apoptosis as detected in (A) BC; (B) N-24, in which the brown globules were abundant and intensive (black arrows); and (C) D-24, in which the brown globules were less prominent compared with the N group (red arrows). (D) Average number of Caspase-3-positive cells of each rat derived from 100 cells of four different fields of view (marked with mean ± SD; magnification, × 200). *P<0.05. BC, blank control group; D-24, dexmedetomidine group 24 h post-ROSC; N-24, normal saline group 24 h post-ROSC; ROSC, return of spontaneous circulation.

Histological and ultrastructural analysis in the rat hippocampus

Histological analysis of hippocampal tissues from the three groups was carried out using H&E staining 24 h post-ROSC; following which the nuclei of cells located in the CA1 region of the hippocampus were examined. Compared with the distinct shape and content of neurocytes from BC group (Fig. 7A; white arrows), cells from the N-24 group exhibited faint nuclear shapes with compact cytoplasm (Fig. 7B; yellow arrows), which indicated that hippocampal neurons were damaged after I/R. Cells from the D-24 group hippocampus displayed visible nuclei and distinct cytoplasm (Fig. 7C; green arrows) compared with N group, which suggested that Dex treatment reduced neural damage following I/R.

Figure 7. Hematoxylin and eosin staining of the rat CA1 region using light microscopy. Hippocampal tissue were isolated from rats 24 h following ROSC in the presence of normal saline or dexmedetomidine. (A) In the BC group, the shape and content of neurocytes were distinct (white arrows). (B) In the N-24 group, the shape of neurocytes was vague with visible shrinkage in the volume and content of neurocytes (yellow arrows). (C) In the D-24 group, the shape, volume and the organelles of neurocytes were more comparable (green arrows) to the BC group in image A. Magnification, ×200; magnified areas are boxed in red. BC, blank control group; D-24, dexmedetomidine group 24 h post-ROSC; N-24, normal saline group 24 h post-ROSC; ROSC, return of spontaneous circulation.

According to the TEM micrographs, the extent of nuclear ultrastructural damage in the hippocampus was less pronounced in the D-24 group compared with the N-24 group. The BC group exhibited a nucleus that appeared normal with an intact nuclear membrane (Fig. 8A), whereas that in the N group was markedly damaged displaying chromatin margination and distorted mitochondria (Fig. 8B). In the D group, these features of damage were less visible (Fig. 8C). In addition, autophagolysosomes (Fig. 8B; black arrows) and heteromorphic mitochondria (Fig. 8B; red arrows) could be observed in the N group. However, little to none of these features were identified in the D group.

Figure 8. Representative electron micrographs of hippocampal neurocytes nuclei. Hippocampal tissue was isolated from the rat hippocampus at 24 h following ROSC. (A) BC group, demonstrating a normal nucleus with an intact nuclear membrane and smooth chromatin; magnification, ×8,000. (B) N-24 group, displaying a markedly damaged nucleus with chromatin margination and condensed nucleoplasm, with autophagosomes (black arrows) and heteromorphic mitochondria (red arrows) in the cytoplasm; magnification, ×12,000. (C) D-24 group, displaying a slightly damaged nucleus with normal nuclear membrane, slightly damaged chromatin and mitochondria (blue arrows) in the cytoplasm; magnification, ×10,000. BC, blank control group; D-24, dexmedetomidine group 24 h post-ROSC; N-24, normal saline group 24 h post-ROSC; ROSC, return of spontaneous circulation.

Discussion

The present study found that Dex administration may induce mild hypothermia, slow down heart rate, attenuate apoptosis of neurocytes and improve neurological function after ROSC following resuscitation from CA. This is supported by histological and ultrastructural observations that Dex reduced damage in the rat hippocampal tissue. Mechanistically, the protective effect of Dex was found to be associated with the downregulation of pro-apoptotic proteins Bax and Caspase-3 with a concomitant upregulation in anti-apoptotic proteins Bcl-2 and HSP70. This is coupled with the finding that the expression of autophagic protein Beclin1 was downregulated in Dex-treated hippocampal tissue.

Dex is an α-2A adrenergic receptor agonist commonly administered to patients as a sedative and analgesic (29). Previous studies have reported Dex to be neuroprotective when combined with hypothermia (30,31). However, few studies have assessed the association between Dex and hypothermia, making the mechanism of this process unclear. Lähdesmäki et al (32) determined that the hypothermic effect of Dex may be abolished if α-2A adrenergic receptor genes were knocked out in mice, which indicated that the activation of α-2A adrenergic receptors, induced by Dex, may inhibit neuronal firing and the release of monoamine neurotransmitters associated with locomotor activity and body temperature. The present study found that the core temperature and heart rate in the group of rats treated with Dex was lower when compared with the saline group in the same post-ROSC environment; which corresponded well with the results from other studies. For example, one previous report suggested that Dex can sustain hypothermia by suppressing muscle shivering (33). It was hypothesized that this effect is caused by the inhibition of neurotransmitter release from sympathetic nerves located within the skeletal muscles by blocking temperature-sensitive vanilloid-type transient receptor potential ion channels (34). In addition, in the sinoatrial node, Dex has been demonstrated to activate cardiac Ca2+-sensitive potassium ion channels in pacemaker cells during repolarization (35), causing a reduction in heart rate.

It was demonstrated in our previous study that mild hypothermia can reduce the level of lactic acid in the blood, alleviate neurocyte apoptosis and improve neurological function in rats that were resuscitated from CA (4). Sato et al (30) found in a rat model of focal cerebral ischemia that short-term neurological outcomes could be improved by a combination of Dex and hypothermia. In the current study, Dex induced hypothermia and improved neurological function in rats after ROSC following CA. However, no difference was found in lactic acid levels between the two groups; this may be due to the collection of arterial blood in 2 h intervals, which did not provide enough time for lactic acid metabolism and excretion. Another possibility was that the duration and severity of hypothermia was not adequate for the elimination of lactic acid, or that Dex may enhance the risk of metabolic acidosis (36).

Zhang et al (37) recently reported that HSP70 conferred cellular protection against ischemic insults and possessed potent anti-apoptotic properties in hippocampal neurons using a traumatic brain injury rat model. To further understand the role of apoptosis and autophagy in neurons after I/R, protein expression levels of Bax, Bcl-2, Caspase-3 and Beclin1 were analyzed in the present study. Bax, Caspase-3 and Beclin1 expression increased after ROSC, suggesting that apoptosis and autophagy were activated by I/R in the hippocampus. However, Dex administration inhibited this increase, subsequently improving neurological function. Therefore, it is possible that Dex may preserve neurological function by reducing neural apoptosis and autophagy following I/R injury. A number of previous studies have demonstrated that Dex can alleviate I/R-induced neurocyte injury either by an intrinsic Bax/Caspase pathway (38) or by inhibiting neuronal autophagy through the upregulation of hypoxia-inducible factor 1α expression (39). Bcl-2 binding to Beclin1 reduces its capacity to activate autophagy without losing its own anti-apoptotic characteristics (40). The results of the present study support the hypothesis that neuronal apoptosis and excessive autophagy may be part of the pathophysiological process in I/R injury following CA, a process that can at least in part be alleviated by Dex.

The present study carries a number of limitations that needs to be addressed in future investigations. The dosage and method of Dex administration would need to be optimized and the mechanism of Dex-induced hypothermia would require further elucidation; both of which can be resolved by in vitro studies. Furthermore, the background luminance of pathological sections was inadequate, making images appear dark in color. In addition, the present study was performed on a rat model in the absence of underlying cardiac-cerebrovascular disease, hampering applicability to human patients.

In the present study, it was found that I/R injury activated Bax, Caspase-3 and Beclin1 expression, which indicated that apoptosis and excessive autophagy may be the main pathological process post-ROSC. The administration of Dex reduced Bax, Caspase-3 and Beclin1 expression levels, induced Bcl-2 and HSP70 expression and hypothermia, and improved neurological function. Therefore, the activation of intracellular apoptosis and autophagy following I/R contributes to neural injury, whereas Dex treatment may induce hypothermia, decrease cellular injury of neurons and improve neurological function.

In conclusion, CA-induced I/R can lead to apoptosis and excessive autophagy in hippocampal neurons. Dex treatment induced hypothermia, in addition to exerting anti-apoptotic and anti-autophagic effects to improve post-resuscitation neurological function after CA. The present study uncovered a potential new treatment strategy for CA recovery.

Acknowledgements

The authors would like to thank the Suzhou Health Commission (Jiangsu, China) for their financial support, the Experimental Center of the Second Affiliated Hospital of Soochow University (Jiangsu, China) for their experimental guidance and the Experimental Center of Suzhou Municipal Hospital and pathology department of Suzhou Vocational Health College (Jiangsu, China) for their technical assistance.

Funding

The current study was supported by a grant from the Science and Technology Project ‘Health of Science and Education’ of Suzhou Province (grant no. KJXW2013026).

Availability of data and materials

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

Authors' contributions

JL proposed the current study and together with LJL, drafted the manuscript. JL and ZL performed the experiments. ZL collected and analyzed experimental data. SY and ZZ modified the manuscript. ZC performed histological and ultrastructural analysis. All authors read and approved the final manuscript for publication.

Ethical approval and consent to participate

The current study was performed according to the exact guidelines and protocols for animal care and use established by the Experimental Center of Suzhou Municipal Hospital (Animal Experiment Permit Number, 120410), and was approved by the Suzhou Municipal Hospital Ethic Committee (Ethical Review Number, KL901008).

Patient consent for publication

Not applicable.

Competing interests

The authors declare that they have no competing interests.

References