Wild Bitter Melon Exerts Anti-Inflammatory Effects by Upregulating Injury-Attenuated CISD2 Expression following Spinal Cord Injury

Kung, Woon-Man; Lin, Chai-Ching; Kuo, Chan-Yen; Juin, Yu-Ching; Wu, Po-Ching; Lin, Muh-Shi

doi:https://doi.org/10.1155/2020/1080521

Behavioural Neurology

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Abstract Introduction Materials and Methods Results Discussion Data Availability Conflicts of Interest Authors’ Contributions Acknowledgments References Copyright Related Articles

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Applications of Theranostics for Detecting and Targeting CNS Injuries and Diseases

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Research Article | Open Access

Volume 2020 | Article ID 1080521 | https://doi.org/10.1155/2020/1080521

Wild Bitter Melon Exerts Anti-Inflammatory Effects by Upregulating Injury-Attenuated CISD2 Expression following Spinal Cord Injury

Woon-Man Kung,¹Chai-Ching Lin,²Chan-Yen Kuo,³Yu-Ching Juin,²Po-Ching Wu,⁴and Muh-Shi Lin^2,5,6,7

Academic Editor: Péter Klivényi

Received04 May 2020

Revised19 Jul 2020

Accepted12 Sept 2020

Published30 Sept 2020

Abstract

Background. Spinal cord injuries (SCIs) induce secondary neuroinflammation through astrocyte reactivation, which adversely affects neuronal survival and eventually causes long-term disability. CDGSH iron sulfur domain 2 (CISD2), which has been reported to be involved in mediating the anti-inflammatory responses, can serve as a target in SCI therapy. Wild bitter melon (WBM; Momordica charantia Linn. var. abbreviata Ser.) contains an anti-inflammatory agent called alpha-eleostearic acid (α-ESA), a peroxisome proliferator-activated receptor-β (PPAR-β) ligand. Activated PPAR-β inhibits the nuclear factor κB (NF-κB) signaling pathway via the inhibition of IκB (inhibitor of NF-κB) degradation. The role of astrocyte deactivation and CISD2 in anti-inflammatory mechanisms of WBM in acute SCIs is unknown. Materials and Methods. A mouse model of SCI was generated via spinal cord hemisection. The SCI mice were administered WBM intraperitoneally (500 mg/kg bodyweight). Lipopolysaccharide- (LPS-) stimulated ALT cells (astrocytes) were used as an in vitro model for studying astrocyte-mediated inflammation post-SCI. The roles of CISD2 and PPAR-β in inflammatory signaling were examined using LPS-stimulated SH-SY5Y cells transfected with si-CISD2 or scramble RNA. Results. WBM mitigated the SCI-induced downregulation of CISD2, PPAR-β, and IκB and upregulation of glial fibrillary acidic protein (GFAP; marker of astrocyte reactivation) in the spinal cord of SCI mice. Additionally, WBM (1 μg/mL) mitigated LPS-induced CISD2 downregulation. Furthermore, SH-SY5Y neural cells with CISD2 knockdown exhibited decreased PPAR-β expression and augmented NF-κB signaling. Conclusion. To the best of our knowledge, this is the first study to report that CISD2 is an upstream modulator of the PPAR-β/NF-κB proinflammatory signaling pathway in neural cells, and that WBM can mitigate the injury-induced downregulation of CISD2 in SCI mice and LPS-stimulated ALT astrocytes.

1. Introduction

Most patients with acute spinal cord injuries (SCIs) exhibit disability. SCIs are associated with expensive and long-term healthcare. The pathophysiology of acute SCIs involves primary and secondary injuries. Primary injury to the spinal cord results in structural damage, disruption of cell membranes and vessels, and degeneration of myelin and axons, which may lead to secondary injury [1]. In SCIs, the pathological mechanisms underlying secondary injuries involve inflammation, free radical production, hyperoxidation, and mitochondrial dysfunction [2, 3]. Extensive injuries to the central nervous system (CNS) may activate the astrocytes, which are the resident immune cells [4, 5]. In response to SCI, astrocytes secrete proinflammatory cytokines and chemokines, thereby inducing a shift in microglial polarization from the beneficial M2 phenotype toward the detrimental M1 phenotype [6–8]. The SCI-induced M1 microglial phenotype is associated with the attenuation of IL-4 expression [9, 10]. The aberrantly activated glial cells (astrocytes and microglia) produce nitric oxide and reactive oxygen species (ROS), which exacerbate the inflammatory response [11]. The activation of inflammatory cascades may be cytotoxic to some neurons and glial cells, which may result in irreversible neurological deficits [12, 13].

Wild bitter melon (WBM) (Momordica charantia Linn. var. abbreviata Ser.) belongs to the family Cucurbitaceae. In Asia and Europe, WBM is used as a medicinal herb to treat various pathological conditions, such as inflammation, hyperglycemia, bacterial infection, and oxidative stress [14]. Mice orally administered WBM exhibit upregulated expression of peroxisome proliferator-activated receptor-α (PPAR-α) and PPAR-γ mRNA, which are involved in hypolipidemic and insulin-sensitizing activities [14]. Additionally, WBM inhibits lipopolysaccharide- (LPS-) induced inflammatory responses in macrophages through the regulation of NF-κB activation [15]. Furthermore, WBM extracts have been demonstrated to scavenge free radicals [16], such as 2,2-diphenyl-1-picrylhydrazyl (DPPH) and hydroxyl radicals [17].

The triglycerides in the seed oils of the family Cucurbitaceae comprise conjugated linolenic acid. Alpha-eleostearic acid (α-ESA, 18 : 3, Δ^{9cis,11trans,13trans}, 9cis, 11trans, 13trans-conjugated linolenic acid) is a linolenic acid, which is widely distributed among the members of the family Cucurbitaceae, including WBM and Momordica charantia (bitter gourd). α-ESA accounts for more than 60% of the total fatty acid composition in bitter gourd seed oil [18]. High-performance liquid chromatography revealed that α-ESA accounts for approximately 19% of the total fatty acid composition of the ethyl acetate extracts. The content of α-ESA in dried and fresh WBM is 7.1 g/kg and 0.42 g/kg, respectively. In WBM seed oil, α-ESA accounts for more than 30% of the total fatty acid content [19].

The ligands of PPAR-β (synonyms: PPAR-δ) include polyunsaturated fatty acids, such as conjugated linoleic acid [20]. α-ESA can be metabolized into conjugated linoleic acid in mice [21] and rats [22]. Therefore, α-ESA can be used as a natural ligand for PPAR-β. Moreover, PPAR-β has been reported to attenuate the production of transforming necrosis factor-α (TNF-α) in cardiomyocyte culture through the inhibition of the NF-κB (nuclear factor κB) signaling pathway [23]. In a mouse model of bleomycin-induced lung injury, the PPAR-β agonist GW0742 inhibited IκB (inhibitor of NF-κB) degradation, thereby consequently deactivating NF-κB [24]. WBM attenuated the generation of inflammatory responses in LPS-stimulated RAW 264.7 macrophages through the inhibition of NF-κB activation [15]. Thus, the interaction between α-ESA and PPAR-β may inhibit IκB degradation and subsequently attenuate NF-κB activation. The pathological mechanisms underlying traumatic SCIs involve mitochondrial oxidative stress and inflammation. Thus, WBM, which exhibits antioxidant and anti-inflammatory activities, may aid the management of acute SCIs.

CDGSH iron sulfur domain 2 (CISD2), known to be associated with aging, has been reported to be involved in conferring protection against mitochondrial dysfunction-induced inflammatory responses and apoptosis. Previously, we had demonstrated that CISD2 was significantly downregulated under conditions of CNS injury and disease, such as aging mouse brain [25] and hemisection injury to the spinal cord in rats [26]. Injury-induced CISD2 downregulation leads to neuroinflammation and mitochondrial dysfunction. Thus, CISD2 can serve as a potential therapeutic target for SCI. This study is aimed at evaluating the role of CISD2 in mediating the anti-inflammatory effects of WBM and the regulatory effects of CISD2 on the PPAR-β/NF-κB signaling pathway using the SCI mouse and in vitro cellular injury models.

2. Materials and Methods

2.1. Extract Preparation and Reagents

WBM dried at low temperature was used to prepare the extract. The WBM samples were ground into a powder and stored at -20°C. WBM powder was incubated with water at room temperature for 24 h with shaking. The suspension was centrifuged at 13,000 g and 4°C for 10 min to remove any residues. The supernatant was freeze-dried, and the lyophilized powder was incubated with ethanol at room temperature for 24 h with shaking. The samples were centrifuged at 13,000 g and 4°C for 10 min, and the supernatant was concentrated under vacuum and stored at -20°C. The concentrated extract was dissolved in absolute alcohol (≧99.8%) before analysis. Absolute alcohol was purchased from Sigma-Aldrich (St. Louis, MO, USA). α-ESA purchased from Cayman Chemical (Ann Arbor, MI, USA) was dissolved in absolute alcohol. LPS (obtained from Escherichia coli serotype 055:B5) was purchased from Sigma-Aldrich (St. Louis, MO, USA; L-2880).

2.2. Animals

Wild-type C57BL/6JNarl mice with an average weight of 22–28 g were obtained from the National Laboratory Animal Center (Taipei, Taiwan). The animals were maintained in a cage for at least 5 days (5 mice per cage) before arrival to our laboratory. The animals had ad libitum access to food and water and were maintained under a 12 h dark/light cycle. The experiments were performed according to the guidelines of the Experimental Animal Laboratory. The animal experiments were approved by the Animal Care and Use Committee at National Ilan University, Yilan, Taiwan (ethical approval code: 105-20).

2.3. Hemisection SCI in Mice

The animal model of acute SCI was generated as described in our previous study [27]. Briefly, the animals were divided into the following three groups: sham control, SCI, and WBM (/group). The mice were anesthetized using isoflurane and placed in a stereotactic apparatus (David Kopf Instruments, Tujunga, CA) to secure the spinal cord. Posterior spinal decompression was performed under a dissecting microscope by performing laminectomy of the ninth to tenth thoracic vertebra without duraplasty. For hemisection of the spinal cord, the guide of the wire knife was positioned along the vertical plane close to the lateral surface in the lower thoracic vertebra of the spinal cord. The knife was turned medially and then extended 1.5 mm. The guide was lifted 4.0 mm to hemitransect the spinal cord. The sham control group underwent surgery, but hemisection of the spinal cord was not performed. The wound was closed in layers using sutures, and recovery was promoted using a heating pad (36.5°C). The animals were starved for 3 h after surgery. Postoperative care included rehydration using subcutaneous saline injection. The mice were returned to their preoperative housing conditions after surgery. A 5 mm section of the spinal cord with the lesion or a similar area in the sham control group was obtained for mRNA extraction and lysate preparation at 8 or 24 h posthemisection (each time point , total for each experimental condition).

2.4. Treating SCI Mice with WBM

The mice in the WBM group were administered WBM intraperitoneally (500 mg/kg body weight; single dose) immediately after SCI. This dosage has been reported to protect mice against inflammation, oxidative stress [28], and hyperglycemia [29]. The mice in the SCI group were administered normal saline intraperitoneally (500 mg/kg body weight) immediately after SCI. The sham operation group was not administered either saline or WBM.

2.5. Neural Cell Lines

The astrocyte cell line (ALT, BCRC 60581) was purchased from the Bioresource Collection and Research Center (BCRC, Hsinchu, Taiwan). ALT cells were cultured in 90% Dulbecco’s modified Eagle’s medium (DMEM) supplemented with 1.5 g/L sodium bicarbonate and 10% fetal bovine serum (FBS). The SH-SY5Y cell line (ATCC, Manassas, VA, USA), derived from human neuroblastoma cells was cultured in DMEM/F-12 supplemented with 10% FBS in an incubator with an atmosphere of 5% CO₂ at 37°C.

2.6. Treatment of LPS-Stimulated ALT Cells with WBM

ALT cells () cultured in a 35 mm dish were stimulated using 20 μg/mL LPS. Next, the cells were treated with 1 μg/mL WBM or 0.28 μg/mL α-ESA for 24 h. Each experiment was performed at least two times with at least three different astrocyte cultures.

2.7. Quantitative Real-Time Polymerase Chain Reaction (qRT-PCR)

Total RNA was extracted from the cultured cells using an extraction buffer (TRIzol/phenol/chloroform). The extracted RNA was reverse transcribed into cDNA using oligo-dT and SuperScript II Reverse Transcriptase (Invitrogen, Carlsbad, CA). The cDNAs were subjected to qRT-PCR to quantify the expression of the target genes. The housekeeping gene cyclophilin was used as an internal control. The PCR conditions were as follows: 25 cycles of 94°C for 1 min (denaturation), 55–60°C for 1 min (annealing), and 72°C for 1 min (extension). The primers used for qRT-PCR are shown in Table 1. The qRT-PCR was performed using SYBR Green on an ABI PRISM 7300 HT Real-Time PCR system (Applied Biosystems, Foster City, CA). The minor groove-binding probes and primers for the detection of target genes and cyclophilin were designed by ABI. The threshold cycle () (the cycle number at which the amount of the amplified target reached a fixed threshold) was determined. The value of the target genes was normalized to that of cyclophilin. Three independent experiments were performed.

2.8. RNA Interference

CISD2 was knocked down in SH-SY5Y cells using small interfering RNA (siRNA). The cells were transfected with CISD2-specific siRNA (si-CISD2) or scrambled siRNA (Silencer® Predesigned siRNA; Ambion, Austin, TX) using Lipofectamine™ 2000 reagent (Invitrogen, Carlsbad, CA). The sequences of si-CISD2 were as follows: 5-GUCCUCUCAUCCUGAAGAATT-3 and 5-UUCUUCAGGAUGAGAGGACTT-3. At 5 h posttransfection, the Lipofectamine 2000-containing medium was replaced with culture medium to allow the cells to recover for 67 h. CISD2 knockdown efficiency was examined using qRT-PCR.

2.9. Immunoblotting

Total protein was extracted from the ALT astrocytes and spinal cord tissues using a lysis buffer (20 mM Tris-HCl, 0.1% sodium dodecyl sulfate (SDS), 0.8% NaCl, and 1% Triton X-100). The protein was subjected to gradient electrophoresis on a 12% gel. The resolved proteins were electroblotted onto a nitrocellulose membrane. The membrane was incubated with a blocking reagent. Next, the membrane was incubated with the following primary antibodies at 4°C for 12 h: anti-IκB alpha (E130) (1 : 2000; ab32518; Abcam, Cambridge, MA, USA), anti-PPAR-β (1 : 2000; ab23673; Abcam), anti-GFAP (1 : 2000; ab7260; Abcam), anti-β-actin (1 : 4000; ab8227; Abcam), and anti-CISD2 (1 : 500; PA5-34545; Thermo Fisher Scientific). The membrane was washed and incubated with goat anti-rabbit IgG (horseradish peroxidase- (HRP-) conjugated secondary antibody) (1 : 5000; 12-348; Merck Millipore) for 1 h. Protein bands were developed using the Immobilon™ Western Chemiluminescent HRP Substrate (WBKLS0500; Merck Millipore). Densitometric analysis of the protein bands was performed using ImageQuant™ LAS 4000 (GE Healthcare Life Sciences).

2.10. Cell Viability

The viability of ALT astrocytes was examined using the 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT) assay. The cells were seeded in a 96-well microplate for 24 h before use. The WBM- or α-ESA-treated ALT cells were incubated with MTT for 4 h. Next, 0.4 N HCl (0.3 mL) in isopropanol was incubated with the mixture overnight to dissolve the formazan crystals. The absorbance of the mixture was measured at 600 nm using an enzyme-linked immunosorbent assay plate reader.

2.11. Statistical Analysis

The variables were subjected to the normality test. Variables exhibiting normal distribution were analyzed using the parametric tests, whereas those exhibiting nonnormal distribution were analyzed using the nonparametric tests. The values in the normality test were >0.05. Therefore, parametric tests were used for comparison of means among the experimental groups.

Independent two-sample -tests were used to compare the means of the two groups. One-way analysis of variance was used to analyze the means of more than two groups.

3. Results

3.1. Effect of WBM and α-ESA on the Viability of ALT Cells

The effects of various concentrations of WBM (0.25–500 μg/mL) and α-ESA (0.07–11.1 μg/mL) on the viability of ALT cells were analyzed using the MTT assay. Compared with the untreated cells, the WBM- (6.25 μg/mL, Figure 1(a)) or α-ESA-treated cells (0.7 μg/mL, Figure 1(c)) exhibited significantly decreased viability. At concentrations of 0.25–6 μg/mL WBM (Figure 1(b)) or 0.07–0.56 μg/mL α-ESA (Figure 1(d)), the viability of ALT cells was greater than 80%. Subsequent in vitro experiments were performed using 1 μg/mL WBM and 0.28 μg/mL α-ESA as at these concentrations, the test agents did not exhibit any cytotoxic effects.

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Figure 1

Cell survival, as measured by MTT assay, of ALT astrocytes following treatment with varying doses of WBM (0.25-500 μg/mL) (a) and α-ESA (0.07-11.1 μg/mL) (c). Concentrations with less cytotoxic effects were determined (>80% of cell viability) at 0.25-6 μg/mL in WBM (b) and 0.07-0.56 μg/mL in α-ESA (d). For in vitro experiments, 1 μg/mL WBM and 0.28 μg/mL α-ESA were selected. Vertical bars indicate the (SEM) (). vs. control. Pair-wise multiple comparisons between groups were determined using the Newman-Keuls method.

3.2. Effect of LPS on the Expression of Proteins Associated with Astrocyte Reactivation and Inflammation

LPS-stimulated ALT cells were used as an in vitro model of cellular injuries. This model recapitulates SCI-associated aberrant astrocyte activation and inflammation [25, 26, 30]. The cells were treated with 20 μg/mL LPS for 24 h and subjected to qRT-PCR and western blotting. The expression of GFAP (, Figure 2(a)), IL-1β (, Figure 2(c)), and IL-6 mRNA (, Figure 2(d)) was significantly upregulated in LPS-stimulated cells compared with that in the control cells. In contrast, the expression of IL-4 (, Figure 2(e)) and CISD2 mRNA (, Figure 2(f)) was significantly downregulated in LPS-stimulated cells when compared with that in the control cells. The expression of GFAP in ALT cells was quantified by western blotting. Compared with that in control cells, the expression of GFAP was significantly upregulated in LPS-stimulated ALT cells (, Figure 2(b)). These findings indicated that the mechanisms underlying injury-induced secondary damage involve aberrant activation of astrocytes, enhanced inflammatory response, and attenuated expression of IL-4 (potentially resulting in impaired polarization of anti-inflammatory M2 microglia) and CISD2.

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Figure 2

Injury-induced CISD2 downregulation, enhanced GFAP mRNA and protein expression, and proinflammation in LPS-challenged ALT astrocytes. WBM can prevent the abovementioned detrimental effects. Results of mRNA expression of GFAP (a), GFAP protein (b), mRNA expression of IL-1β (c), IL-6 (d), IL-4 (e), and CISD2 (f) in ALT cells with or without administration of WBM and α-ESA. Vertical bars indicate the (SEM) of mRNA expression (). vs. control,vs. control,vs. control, ^#, ^##, and ^###indicate a significant difference. Pair-wise multiple comparisons between groups were performed using the Newman-Keuls method.

3.3. WBM and α-ESA Attenuated LPS-Induced Changes in ALT Astrocytes

Next, the effects of WBM and α-ESA on the expression of IL-4 and CISD2 in LPS-stimulated ALT cells were evaluated. ALT cells were treated with 20 μg/mL LPS, 20 μg/mL LPS, and 1 μg/mL WBM, or 20 μg/mL LPS and 0.28 μg/mL α-ESA for 24 h, and subjected to qRT-PCR and western blotting.

Compared with LPS-stimulated ALT cells, ALT cells treated with WBM or α-ESA in the background of LPS stimulation exhibited significant downregulation of GFAP mRNA (both , Figure 2(a)) as well as protein levels (both , Figure 2(b)). Additionally, the expression of IL-1β ( or , respectively, Figure 2(c)) and IL-6 mRNA ( or , respectively, Figure 2(d)) in ALT cells treated with WBM or α-ESA in the background of LPS stimulation was lower than that in LPS-stimulated ALT cells. Moreover, the expression of IL-4 (both , Figure 2(e)) and CISD2 mRNA (both , Figure 2(f)) in ALT cells treated with WBM or α-ESA in the background of LPS stimulation was lower than that in LPS-stimulated ALT cells. These findings indicated that α-ESA is the bioactive component, and it is responsible for the anti-inflammatory effect of WBM. We hypothesized that the mechanism underlying the anti-inflammatory activity of WBM in LPS-stimulated ALT cells involves astrocyte deactivation, proinflammatory cytokine attenuation, and enhanced IL-4 and CISD2 expression.

3.4. Effect of CISD2 Knockdown on PPAR-β Expression and Inflammatory Response in the SH-SY5Y Cells

CISD2 has been reported to inhibit inflammation through the regulation of upstream components of the NF-κB signaling pathway [39]. Attenuation of CISD2 promotes inflammation in various CNS-associated conditions, such as aging [20], injuries, and degeneration [19]. α-ESA, a bioactive anti-inflammatory compound in WBM, serves as a PPAR-β ligand. Thus, α-ESA suppresses NF-κB signaling and downstream cytokine production by inhibiting IκB degradation. Next, the effects of WBM and α-ESA on the expression of CISD2 and PPAR-β, which are the upstream effectors of the NF-κB signaling pathway, were examined. SH-SY5Y cells are recognized as a well-established in vitro model to evaluate neural function. In this study, SH-SY5Y cells were transfected with si-CISD2 to knockdown CISD2. Previous studies have reported that si-CISD2 achieved approximately 60% knockdown efficiency in SH-SY5Y cells [26].

The results of qRT-PCR are shown in Figure 3(a). The band intensities reproducibly confirmed the anti-inflammatory effect of CISD2. Compared with the scramble siRNA-transfected cells, si-CISD2-transfected cells exhibited significant upregulation of NF-κB p105 (, Figure 3(b)), COX-2 (, Figure 3(c)), and RANTES mRNA (, Figure 3(d)). Furthermore, the expression of PPAR-β mRNA in si-CISD2-transfected cells was significantly lower than that in the control cells (untreated with si-CISD2) (, Figure 3(e)). These findings indicated that CISD2 acts on the upstream components of the PPAR-β/NF-κB signaling pathway, and that it is involved in NF-κB-mediated aberrant activation of astrocytes and proinflammatory cascades.

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Figure 3

Knockdown of CISD2 expression in neural cells significantly influenced mRNA expression levels in PPAR-β, indicating upstream regulation of CISD2 on PPAR-β (a). mRNA levels of NF-κB, COX-2, and RANTES were determined by semiquantitative RT-PCR in neural cells with or without si-CISD2 transfection. The results shown are from one of the experiments that were repeated for at least 3 times. Quantification of relative band intensity of semiquantitative RT-PCR showed that CISD2 knockdown in neural cells led to enhanced mRNA expression levels in NF-κB (b) and downstream proinflammatory mediators including COX-2 (c) and RANTES (d). (e) Results of real-time qRT-PCR for mRNA levels of PPAR-β in neural cells with or without si-CISD2 transfection. Vertical bars indicate the (SEM) of mRNA expression (). and indicate a statistically significant difference between the control and si-CISD2 groups using independent two-sample -tests.

3.5. Effects of WBM on SCI Mice

Next, the effect of WBM on the expression of CISD2 in mice with hemisection SCI was evaluated. The SCI mice were intraperitoneally administered WBM (500 mg/kg body weight) or normal saline. At 24 h post-SCI, qRT-PCR was performed to analyze the expression of genes involved in astrocyte-mediated inflammation, such as GFAP, IL-4, and CISD2, in the damaged spinal cord. Compared with the sham control group, the SCI group exhibited upregulation of GFAP (, Figure 4(a)), IL-1β (, Figure 4(b)), and IL-6 mRNA (, Figure 4(c)) and downregulation of IL-4 (, Figure 4(d)) and CISD2 mRNA (, Figure 4(e)). These findings suggested that SCIs result in inhibited IL-4 and CISD2 expression, aberrant astrocyte activation, and enhanced inflammation [26].

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Figure 4

Traumatic insults upregulated GFAP and neuroinflammatory mediators and downregulated CISD2 mRNA expression in vivo 24 h after spinal cord hemisection in mice. WBM can in vivo rescue the abovementioned detrimental effects. Results of mRNA expression of GFAP (a), IL-1β (b), IL-6 (c), IL-4 (d), and CISD2 (e) for 3 conditions. Vertical bars indicate the (SEM) of mRNA expression (). vs. control, vs. control, ^##, and ^### indicate a significant difference. Pair-wise multiple comparisons between groups were performed using the Newman-Keuls method.

Compared with the SCI group, the WBM group exhibited downregulation of GFAP (, Figure 4(a)), IL-1β (, Figure 4(b)), and IL-6 mRNA (, Figure 4(c)) and upregulation of IL-4 (, Figure 4(d)) and CISD2 mRNA (, Figure 4(e)). Thus, the anti-inflammatory effects of WBM in SCI mice may involve inhibition of astroglial activity, attenuation of glia-mediated inflammatory responses, and enhanced production of IL-4 (which potentially enhances the M2 microglial population) and CISD2.

3.6. Anti-Inflammatory Mechanisms of WBM in SCI Mice

Finally, we demonstrated that the CISD2/PPAR-β/NF-κB signaling pathway is involved in mediating the anti-inflammatory effect of WBM in mice with hemisection SCI. Western blotting was performed to evaluate the therapeutic effects of WBM with respect to the mouse spinal cord with or without SCI.

No detrimental effects were observed at 8 h post-SCI (Figures 5(a), 5(c), and 5(d)). Moreover, the expression of PPAR-β (, Figure 5(b)) and IκB proteins (, Figure 5(c)) in the injured spinal cord of the WBM group was upregulated compared to that in the injured spinal cord of the SCI group. However, WBM-mediated downregulation of GFAP and upregulation of CISD2 in mice with SCI were nonsignificant (Figures 5(a) and 5(d), respectively). The effects of WBM on the expression of GFAP and CISD2 were significant at 24 h post-SCI.

Figure 5

WBM abolished injury-triggered GFAP and attenuated injury-downregulated CISD2, PPAR-β, and IκB protein expression in mice 24 h following spinal cord hemisection in vivo. (a–d) In vivo mouse model of SCI. Results of protein expression of CISD2 (a), PPAR-β (b), IκB (c), and GFAP (d) for 3 conditions 8 h after SCI. (e–h) Results of protein expression of CISD2 (e), PPAR-β (f), IκB (g), and GFAP (h) for 3 conditions 24 h after SCI. The lower panel indicates representative immunoblot of the proposed protein expression, and β-actin (42 kDa) serves as an internal control. The results shown were from one of the experiments that were repeated for at least 3 times. The upper panel indicates the of the proposed protein/β-actin band intensity in ratio to the control group. Anti-inflammatory effects of WBM on SCI can be postulated as CISD2 preservation, and the potential upstream regulation of CISD2 on PPAR-β, subsequent IκB stabilization, and therefore, NF-κB inhibition. Vertical bars indicate the (SEM) of protein expression (). vs. control, vs. control, vs. control, ^#, ^##, and ^### indicate a significant difference. Pair-wise multiple comparisons between groups were performed using the Newman-Keuls method.

At 24 h post-SCI, compared with the sham group, the SCI group exhibited significant upregulation of GFAP (, Figure 5(h)) and significant downregulation of PPAR-β (, Figure 5(f)), IκB (, Figure 5(g)), and CISD2 proteins (, Figure 5(e)) in the injured spinal cord. Furthermore, compared with the SCI group, the WBM group exhibited significant downregulation of GFAP (, Figure 5(h)) and significant upregulation of PPAR-β (, Figure 5(f)), IκB (, Figure 5(g)), and CISD2 proteins (, Figure 5(e)) in the injured spinal cord. These in vivo findings suggested that WBM mitigated the SCI-induced downregulation of CISD2 at mRNA and protein levels, and inhibited the PPAR-β/IκB/NF-κB signaling pathway, which was in agreement with the in vitro results.

4. Discussion

Various CNS-associated conditions, such as aging, neurodegeneration, and traumatic brain injury or SCIs are associated with inflammation [31–33] and mitochondrial dysfunction [34, 35]. Activated glial cell-mediated inflammation can contribute to mitochondrial dysfunction, which impairs mitochondrial dynamics and membrane permeabilization and promotes ROS production [36, 37]. Mitochondrial dysfunction can exacerbate the inflammatory response [38]. Prolonged inflammation and mitochondrial dysfunction may lead to irreversible neuronal deficits.

CISD2, an outer mitochondrial membrane protein, is reported to be involved in the maintenance of mitochondrial integrity and calcium metabolism, as well as in the inhibition of apoptosis. It is involved in maintaining the calcium pool in the endoplasmic reticulum (ER), so as to prevent Ca²⁺ surge [39]. Compared with the wild-type mice, the CISD2 knockout mice exhibit increased Ca²⁺ levels in the ER and cytoplasm [40], mitochondrial dysfunction, and enhanced cell death [41]. CISD2 can bind BCL2 and promote the formation of the BCL2-BECN1 complex, which inhibits Beclin 1, a promoter of apoptosis [42].

In addition to mitochondrial dysfunction, CISD2 mitigates CNS injury-induced inflammatory response. Aging, neurodegeneration, and trauma are associated with downregulated CISD2 expression, which enhances the inflammatory response and exacerbates mitochondrial dysfunction [25, 26]. Therefore, therapeutic targeting of CISD2 can aid in preventing the exacerbation of inflammation and mitochondrial dysfunction.

NF-κB signaling is active in the cytoplasm and mitochondrial intermembranous space. The NF-κB signaling pathway is involved in mediating phenomenon, such as mitochondrial dynamics and respiratory electron transport chain. Aberrant activation of NF-κB promotes mitochondrial dysfunction and apoptosis [43]. Additionally, the mechanisms underlying inflammation and mitochondrial dysfunction associated with aging, neurodegenerative disease, and head trauma or acute SCIs may involve aberrant NF-κB activation. Further studies are needed to elucidate the role of CISD2 in regulating the NF-κB signaling pathway.

BCL2 and NF-κB are the upstream targets of CISD2 [44]. In this study, we demonstrated that CISD2 regulates the upstream effectors (PPAR-β) of the PPAR-β/IκB/NF-κB signaling pathway. Additionally, the findings of this study indicated that the anti-inflammatory mechanism of CISD2 involves inhibition of NF-κB activity. Furthermore, CISD2 is an outer mitochondrial membrane structural protein that may be degraded during the pathological process of primary injury (in acute trauma) or secondary injury (in chronic inflammation) associated with CNS injury or disease. CISD2 is downregulated under nonstressed and injured conditions [25]. Insult-induced CISD2 downregulation results in the inhibition of NF-κB activity in the cytoplasm and mitochondria. This explains the wide range of harmful effects, including enhanced inflammation and mitochondrial dysfunction, associated with injury-induced CISD2 downregulation.

Previously, we had demonstrated that curcumin mitigated injury-induced CISD2 downregulation, suggesting that curcumin exerts a protective effect against inflammation and mitochondrial dysfunction in mice with hemisection SCI [26] and aged mice (104 weeks) [25]. CISD2 deficiency enhances the expression of iNOS and RANTES, which contributes to mitochondrial dysfunctions, such as low DeltaPsi(m) levels, high ROS levels, and augmented apoptosis, which are mitigated upon curcumin treatment [25]. In this study, WBM mitigated the injury-induced downregulation of CISD2, which inhibited the aberrant activation of glia and proinflammatory cascades in SCI-hemisected mice and LPS-stimulated ALT cells. WBM enhanced the expression of CISD2, PPAR-β, and IκB proteins in the spinal cord of SCI mice. Hence, we hypothesized that WBM upregulates CISD2, which negatively regulates the PPAR-β/IκB/NF-κB signaling pathway and alleviates inflammation and mitochondrial dysfunction through NF-κB. Pharmacological agents that target CISD2 can be considered for treating CNS injury or disease. Further studies are needed to elucidate the role of NF-κB activation in CISD2-mediated alleviation of inflammation and mitochondrial dysfunction.

This study has several limitations. The anti-inflammatory effects of WBM were evaluated based on the expression of CISD2 and attenuation of aberrant glial activation in SCI mice. However, the mechanism underlying injury-induced aberrant glial activation involves astrocyte-microglia interaction. In this study, WBM mitigated the injury-induced upregulation of GFAP in SCI mice and LPS-stimulated ALT cells. This indicated that WBM deactivated the astrocytes. WBM mitigated SCI-induced downregulation of IL-4 in mice with SCI. The loss of IL-4 promotes microglial polarization from M2 to M1 phenotype in IL-4 knockout mice [10]. Thus, WBM can potentially enhance the levels of anti-inflammatory M2 microglia in SCI mice. Further in vivo studies are needed to examine the mechanism underlying WBM-mediated microglial polarization in SCIs. Furthermore, si-CISD2 transfection revealed that the anti-inflammatory effects of CISD2 were associated with the regulation of PPAR-β, which positively regulates IκB, an inhibitor of NF-κB. Hence, we hypothesized that the injury-induced downregulation of CISD2 inhibited NF-κB activity in the cytoplasm and mitochondria, which resulted in enhanced inflammation and mitochondrial dysfunction. Future studies must elucidate the detailed mechanism underlying CISD2-mediated regulation of NF-κB and glial activation. However, the findings of this study indicated that CISD2 regulates inflammation and mitochondrial dysfunction via the inhibition of NF-κB.

In conclusion, WBM exerted its anti-inflammatory effects through the upregulation of CISD2 in SCI mice and LPS-stimulated ALT cells. CISD2 exhibits protective activity in SCI mice via NF-κB downregulation and astrocyte deactivation.

Data Availability

Answer: yes. Comment: the data used to support the findings of this study are included within the article.

Conflicts of Interest

No competing financial interests exist.

Authors’ Contributions

Woon-Man Kung contributed in writing the original draft of the manuscript as well as in formal analysis. Chai-Ching Lin contributed in supervision, investigation, and formal analysis. Chan-Yen Kuo contributed in project administration and validation. Yu-Ching Juin contributed in project administration and methodology. Po-Ching Wu contributed resources as well as in supervision and investigation. Muh-Shi Lin contributed in funding acquisition; writing the original draft of the manuscript; writing, reviewing, and editing the final version of the manuscript; and in conceptualization.

Acknowledgments

Part of the information reported in Results was referenced from the master thesis of Yu-Ching Juin at the National Ilan University, Yilan, Taiwan. This work was supported by grants from the Kuang Tien General Hospital, Taiwan (Kuang Tien 105-07 and 106-12).

References

B. K. Kwon, W. Tetzlaff, J. N. Grauer, J. Beiner, and A. R. Vaccaro, “Pathophysiology and pharmacologic treatment of acute spinal cord injury,” The Spine Journal, vol. 4, no. 4, pp. 451–464, 2004.
View at: Publisher Site | Google Scholar
J. R. Bethea and W. D. Dietrich, “Targeting the host inflammatory response in traumatic spinal cord injury,” Current Opinion in Neurology, vol. 15, no. 3, pp. 355–360, 2002.
View at: Publisher Site | Google Scholar
J. D. Houle and A. Tessler, “Repair of chronic spinal cord injury,” Experimental Neurology, vol. 182, no. 2, pp. 247–260, 2003.
View at: Publisher Site | Google Scholar
S. J. Davies, P. M. Field, and G. Raisman, “Regeneration of cut adult axons fails even in the presence of continuous aligned glial pathways,” Experimental Neurology, vol. 142, no. 2, pp. 203–216, 1996.
View at: Publisher Site | Google Scholar
K. S. Hung, S. L. Hwang, C. L. Ling et al., “Calpain inhibitor inhibits p35-p25-Cdk5 activation, decreases tau hyperphosphorylation, and improves neurological function after spinal cord hemisection in rats,” Journal of Neuropathology and Experimental Neurology, vol. 64, no. 1, pp. 15–26, 2005.
View at: Publisher Site | Google Scholar
Y. Luo, M. A. Berman, Q. Zhai et al., “RANTES stimulates inflammatory cascades and receptor modulation in murine astrocytes,” Glia, vol. 39, no. 1, pp. 19–30, 2002.
View at: Publisher Site | Google Scholar
C. H. Tator and M. G. Fehlings, “Review of the secondary injury theory of acute spinal cord trauma with emphasis on vascular mechanisms,” Journal of Neurosurgery, vol. 75, no. 1, pp. 15–26, 1991.
View at: Publisher Site | Google Scholar
W. Liu, Y. Tang, and J. Feng, “Cross talk between activation of microglia and astrocytes in pathological conditions in the central nervous system,” Life Sciences, vol. 89, no. 5-6, pp. 141–146, 2011.
View at: Publisher Site | Google Scholar
G. Volpin, M. Cohen, M. Assaf, T. Meir, R. Katz, and S. Pollack, “Cytokine levels (IL-4, IL-6, IL-8 and TGFβ) as potential biomarkers of systemic inflammatory response in trauma patients,” International Orthopaedics, vol. 38, no. 6, pp. 1303–1309, 2014.
View at: Publisher Site | Google Scholar
X. Liu, J. Liu, S. Zhao et al., “Interleukin-4 is essential for microglia/macrophage M2 polarization and long-term recovery after cerebral ischemia,” Stroke, vol. 47, no. 2, pp. 498–504, 2016.
View at: Publisher Site | Google Scholar
S. Li, L. Wang, M. A. Berman, Y. Zhang, and M. E. Dorf, “RNAi screen in mouse astrocytes identifies phosphatases that regulate NF-κB signaling,” Molecular Cell, vol. 24, no. 4, pp. 497–509, 2006.
View at: Publisher Site | Google Scholar
K. S. Hung, S. H. Tsai, T. C. Lee, J. W. Lin, C. K. Chang, and W. T. Chiu, “Gene transfer of insulin-like growth factor-I providing neuroprotection after spinal cord injury in rats,” Journal of Neurosurgery. Spine, vol. 6, no. 1, pp. 35–46, 2007.
View at: Publisher Site | Google Scholar
R. J. Hurlbert, “Strategies of medical intervention in the management of acute spinal cord injury,” Spine, vol. 31, Supplement, pp. S16–S21, 2006.
View at: Publisher Site | Google Scholar
C. Y. Chao, M. C. Yin, and C. J. Huang, “Wild bitter gourd extract up-regulates mRNA expression of PPARα, PPARγ and their target genes in C57BL/6J mice,” Journal of Ethnopharmacology, vol. 135, no. 1, pp. 156–161, 2011.
View at: Publisher Site | Google Scholar
C. K. Lii, H. W. Chen, W. T. Yun, and K. L. Liu, “Suppressive effects of wild bitter gourd (Momordica charantia Linn. var. abbreviata ser.) fruit extracts on inflammatory responses in RAW264.7 macrophages,” Journal of Ethnopharmacology, vol. 122, no. 2, pp. 227–233, 2009.
View at: Publisher Site | Google Scholar
Y. L. Lu, Y. H. Liu, J. H. Chyuan, K. T. Cheng, and W. L. Liang, “Antioxidant activities of different wild bitter gourd (Momordica charantia L. var. abbreviata Seringe) cultivars,” Botanical Studies, vol. 53, pp. 207–214, 2012.
View at: Google Scholar
S. J. Wu and L. T. Ng, “Antioxidant and free radical scavenging activities of wild bitter melon (Momordica charantia Linn. var. abbreviata Ser.) in Taiwan,” LWT-Food Science and Technology, vol. 41, no. 2, pp. 323–330, 2008.
View at: Publisher Site | Google Scholar
R. Rawat, X. H. Yu, M. Sweet, and J. Shanklin, “Conjugated fatty acid synthesis: residues 111 and 115 influence product partitioning of Momordica charantia conjugase,” The Journal of Biological Chemistry, vol. 287, no. 20, pp. 16230–16237, 2012.
View at: Publisher Site | Google Scholar
C. Y. Chuang, C. Hsu, C. Y. Chao, Y. S. Wein, Y. H. Kuo, and C. J. Huang, “Fractionation and identification of 9c, 11t, 13t-conjugated linolenic acid as an activator of PPARα in bitter gourd (Momordica charantia L.),” Journal of Biomedical Science, vol. 13, no. 6, pp. 763–772, 2006.
View at: Publisher Site | Google Scholar
Y. Liu, J. K. Colby, X. Zuo, J. Jaoude, D. Wei, and I. Shureiqi, “The role of PPAR-δ in metabolism, inflammation, and cancer: many characters of a critical transcription factor,” International Journal of Molecular Sciences, vol. 19, no. 11, p. 3339, 2018.
View at: Publisher Site | Google Scholar
G. F. Yuan, A. J. Sinclair, C. Q. Zhou, and D. Li, “α-Eleostearic acid is more effectively metabolized into conjugated linoleic acid than punicic acid in mice,” Journal of the Science of Food and Agriculture, vol. 89, no. 6, pp. 1006–1011, 2009.
View at: Publisher Site | Google Scholar
T. Tsuzuki, Y. Tokuyama, M. Igarashi et al., “α-Eleostearic acid (9Z11E13E-18:3) is quickly converted to conjugated linoleic acid (9Z11E-18:2) in rats,” The Journal of Nutrition, vol. 134, no. 10, pp. 2634–2639, 2004.
View at: Publisher Site | Google Scholar
G. Ding, L. Cheng, Q. Qin, S. Frontin, and Q. Yang, “PPARδ modulates lipopolysaccharide-induced TNFα inflammation signaling in cultured cardiomyocytes,” Journal of Molecular and Cellular Cardiology, vol. 40, no. 6, pp. 821–828, 2006.
View at: Publisher Site | Google Scholar
M. Galuppo, R. di Paola, E. Mazzon et al., “GW0742, a high affinity PPAR-β/δ agonist reduces lung inflammation induced by bleomycin instillation in mice,” International Journal of Immunopathology and Pharmacology, vol. 23, no. 4, pp. 1033–1046, 2010.
View at: Publisher Site | Google Scholar
C. C. Lin, T. H. Chiang, Y. Y. Sun, and M. S. Lin, “Protective effects of CISD2 and influence of curcumin on CISD2 expression in aged animals and inflammatory cell model,” Nutrients, vol. 11, no. 3, p. 700, 2019.
View at: Publisher Site | Google Scholar
C. C. Lin, T. H. Chiang, W. J. Chen, Y. Y. Sun, Y. H. Lee, and M. S. Lin, “CISD2 serves a novel role as a suppressor of nitric oxide signalling and curcumin increases CISD2 expression in spinal cord injuries,” Injury, vol. 46, no. 12, pp. 2341–2350, 2015.
View at: Publisher Site | Google Scholar
M. S. Lin, Y. H. Lee, W. T. Chiu, and K. S. Hung, “Curcumin provides neuroprotection after spinal cord injury,” The Journal of Surgical Research, vol. 166, no. 2, pp. 280–289, 2011.
View at: Publisher Site | Google Scholar
K. H. Lu, H. C. Tseng, C. T. Liu, C. J. Huang, J. H. Chyuan, and L. Y. Sheen, “Wild bitter gourd protects against alcoholic fatty liver in mice by attenuating oxidative stress and inflammatory responses,” Food & Function, vol. 5, no. 5, pp. 1027–1037, 2014.
View at: Publisher Site | Google Scholar
X.-Q. Yuan, X. Gu, J. Tang, and J. Wasswa, “Hypoglycemic effect of semipurified peptides from Momordica charantia L. var. Abbreviata Ser. in alloxan-induced diabetic mice,” Journal of Food Biochemistry, vol. 32, no. 1, pp. 107–121, 2008.
View at: Publisher Site | Google Scholar
M. S. Lin, Y. Y. Sun, W. T. Chiu et al., “Curcumin attenuates the expression and secretion of RANTES after spinal cord injury in vivo and lipopolysaccharide-induced astrocyte reactivation in vitro,” Journal of Neurotrauma, vol. 28, no. 7, pp. 1259–1269, 2011.
View at: Publisher Site | Google Scholar
N. J. Maragakis and J. D. Rothstein, “Mechanisms of disease: astrocytes in neurodegenerative disease,” Nature Clinical Practice. Neurology, vol. 2, no. 12, pp. 679–689, 2006.
View at: Publisher Site | Google Scholar
S. Hickman, S. Izzy, P. Sen, L. Morsett, and J. el Khoury, “Microglia in neurodegeneration,” Nature Neuroscience, vol. 21, no. 10, pp. 1359–1369, 2018.
View at: Publisher Site | Google Scholar
A. Ravari, T. Mirzaei, D. Kennedy, and M. Kazemi Arababadi, “Chronoinflammaging in Alzheimer: a systematic review on the roles of toll like receptor 2,” Life Sciences, vol. 171, pp. 16–20, 2017.
View at: Publisher Site | Google Scholar
A. Navarro and A. Boveris, “Brain mitochondrial dysfunction in aging, neurodegeneration, and Parkinson’s disease,” Frontiers in Aging Neuroscience, vol. 2, p. 34, 2010.
View at: Publisher Site | Google Scholar
N. Sun, R. J. Youle, and T. Finkel, “The mitochondrial basis of aging,” Molecular Cell, vol. 61, no. 5, pp. 654–666, 2016.
View at: Publisher Site | Google Scholar
J. van Horssen, P. van Schaik, and M. Witte, “Inflammation and mitochondrial dysfunction: A vicious circle in neurodegenerative disorders?” Neuroscience letters, vol. 710, article 132931, 2019.
View at: Publisher Site | Google Scholar
R. L. Hunter, N. Dragicevic, K. Seifert et al., “Inflammation induces mitochondrial dysfunction and dopaminergic neurodegeneration in the nigrostriatal system,” Journal of Neurochemistry, vol. 100, no. 5, pp. 1375–1386, 2007.
View at: Publisher Site | Google Scholar
M. N. Valcárcel-Ares, R. R. Riveiro-Naveira, C. Vaamonde-García et al., “Mitochondrial dysfunction promotes and aggravates the inflammatory response in normal human synoviocytes,” Rheumatology (Oxford), vol. 53, no. 7, pp. 1332–1343, 2014.
View at: Publisher Site | Google Scholar
N. C. Chang, M. Nguyen, J. Bourdon et al., “Bcl-2-associated autophagy regulator Naf-1 required for maintenance of skeletal muscle,” Human Molecular Genetics, vol. 21, no. 10, pp. 2277–2287, 2012.
View at: Publisher Site | Google Scholar
N. C. Chang, M. Nguyen, and G. C. Shore, “BCL2-CISD2: An ER complex at the nexus of autophagy and calcium homeostasis?” Autophagy, vol. 8, no. 5, pp. 856-857, 2014.
View at: Publisher Site | Google Scholar
Y. F. Chen, C. H. Kao, Y. T. Chen et al., “Cisd2 deficiency drives premature aging and causes mitochondria-mediated defects in mice,” Genes & Development, vol. 23, no. 10, pp. 1183–1194, 2009.
View at: Publisher Site | Google Scholar
R. Kang, H. J. Zeh, M. T. Lotze, and D. Tang, “The Beclin 1 network regulates autophagy and apoptosis,” Cell Death and Differentiation, vol. 18, no. 4, pp. 571–580, 2011.
View at: Publisher Site | Google Scholar
B. C. Albensi, “What is nuclear factor kappa B (NF-κB) doing in and to the mitochondrion?” Frontiers in Cell and Development Biology, vol. 7, p. 154, 2019.
View at: Publisher Site | Google Scholar
B. Chen, S. Shen, J. Wu et al., “CISD2 associated with proliferation indicates negative prognosis in patients with hepatocellular carcinoma,” International Journal of Clinical and Experimental Pathology, vol. 8, no. 10, pp. 13725–13738, 2015.
View at: Google Scholar

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Copyright © 2020 Woon-Man Kung et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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