Upregulation of miR-34a by Inhibition of IRE1<i>α</i> Has Protective Effect against A<i>β</i>-Induced Injury in SH-SY5Y Cells by Targeting Caspase-2

Li, Qianqian; Liu, Tingjiao; Yang, Shanshan; Zhang, Zhongling

doi:https://doi.org/10.1155/2019/2140427

Oxidative Medicine and Cellular Longevity

On this page

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

Research Article | Open Access

Volume 2019 | Article ID 2140427 | https://doi.org/10.1155/2019/2140427

Upregulation of miR-34a by Inhibition of IRE1α Has Protective Effect against Aβ-Induced Injury in SH-SY5Y Cells by Targeting Caspase-2

Qianqian Li,¹Tingjiao Liu,¹Shanshan Yang,¹and Zhongling Zhang¹

Academic Editor: Jeferson L. Franco

Received06 Mar 2019

Accepted21 Apr 2019

Published02 Jun 2019

Abstract

Background. Neurotoxicity induced by the amyloid-β (Aβ) peptide is one of the most important pathological mechanisms of Alzheimer’s disease (AD). Based on accumulating evidence in AD research, both endoplasmic reticulum stress (ER stress) and alterations in the microRNA (miRNA) network contribute to the pathogenesis of the disease, making them potential therapeutic targets for AD. The present study was performed to investigate whether miR-34a and the inositol-requiring enzyme 1 (IRE1) are involved in the regulation of Aβ-induced cytotoxicity. Methods. Human neuroblastoma SH-SY5Y cells were treated with Aβ1-40. Cell viability was assessed by the MTT assay. The integrity of the plasma membrane was assessed by LDH release. The expression levels of XBP1s, IRE1α, p-IRE1α, and Caspase-2 were detected by Western blot analysis. Spliced-XBP1 mRNA and miR-34a were detected by reverse transcription- (RT-) PCR and quantitative real-time PCR, respectively. Caspase-2 activity was measured using the Caspase-2 cellular activity assay kit. The IRE1 inhibitor (STF-083010) was used to determine the role of IRE1α on miR-34a expression. SH-SY5Y cells were transfected with miR-34a mimics to assess the role of miR-34a on the activation of Caspase-2 and the viability of Aβ-exposed SH-SY5Y cells. Results. We showed that Aβ caused concentration- and duration-dependent death of SH-SY5Y cells. The expression levels of XBP1s, p-IRE1α, and Caspase-2 were increased, along with a corresponding decrease in the miR-34a levels in Aβ-exposed SH-SY5Y cells. The IRE1 inhibitor (STF-083010) upregulated the expression of miR-34a and suppressed the activation of Caspase-2, effectively alleviating the Aβ-induced death of SH-SY5Y cells. Transfection studies show that miR-34a mimics inhibit the expression of Caspase-2 and restore the viability of Aβ-exposed SH-SY5Y cells. Conclusion. Aβ peptide induced downregulation of miR-34a through the activation of IRE1α, which may induce cytotoxicity by targeting Caspase-2. Upregulation of miR-34a by inhibition of IRE1α has protective effects against Aβ-induced injury in SH-SY5Y cells.

1. Introduction

Alzheimer’s disease (AD) is a chronic and progressive neurodegenerative disease of the central nervous system. It is characterized by extracellular aggregates of amyloid-β (Aβ) peptide in senile plaques [1]. Previous studies provide strong evidence that Aβ plays a central role in the pathogenesis of AD [2–4].

The endoplasmic reticulum (ER) is responsible for controlling proper protein synthesis, posttranslational modifications, and protein folding, which is crucial for cell survival. ER stress occurs when the accumulation of nonfolded or misfolded proteins exceeds the processing capacity of the ER under physiological conditions [5]. When cells fail to recover from ER stress, the unfolded protein response (UPR) triggers apoptosis [6]. Inositol-requiring enzyme 1 (IRE1), a transmembrane protein that has both Ser/Thr protein kinases and endoribonuclease activities, is one of the major ER sensors that responds to the aggregation of unfolded proteins [7, 8]. Two types of IRE1 are expressed in mammals, IRE1α and IRE1β. IRE1α is widely expressed in a variety of cells, whereas IRE1β is only expressed in the intestine and lung. Activation of IRE1α involves its dimerization, oligomerization, and autophosphorylation. Upon activation, IRE1α excises a 26-base intron from the x-box binding protein 1 (XBP1) mRNA, producing an active transcription factor (XBP1s) [9–12]. IRE1α and XBP1s are key molecules regulating ER stress; the activation of IRE1α and the upregulation of the XBP1s expression are often used as markers of the UPR to induce ER stress [13]. However, IRE1α acts as a double-edged sword. If restoring ER homeostasis fails, IRE1α initiates apoptosis by regulating a large list of substrates, which may eventually induce cell death [14, 15].

MicroRNAs (miRNAs), a type of small noncoding mRNA containing approximately 22 nucleotides, regulate the expression of at least 30% of all genes through binding of the 3-untranslated region of their target mRNAs, leading to their inhibition of translation or destabilization [16–18]. miR-34a, a gene product of chromosomal locus 1p36.23, is particularly pronounced in the central nervous system (CNS) [19]. Increasing evidence shows that miR-34a dysfunction may contribute to pathologies of the CNS [20, 21]. IRE1α has recently been shown to cleave miR-34a, resulting in activation of Caspase-2, which may help initiate apoptosis [22, 23]. Based on previous studies, we explored whether there is activated IRE1α and abnormal expression of miR-34a in Aβ-treated SH-SY5Y cells to clarify the role of the IRE1α/miR-34a pathway in Aβ-induced cytotoxicity.

2. Materials and Methods

2.1. Reagents

The Aβ1-40 peptide was obtained from Sigma-Aldrich (St. Louis, MO, USA). STF-083010, a specific IRE1α I endonuclease inhibitor, was bought from Sigma-Aldrich and was prepared fresh in a dark room with DMSO for a 25 mM stock solution. The RNA Fast Isolation kit and M-MLV Reverse Transcriptase were obtained from BioTeke Corporation (Beijing, China). The SYBR Green PCR Kit was purchased from Solarbio Science & Technology (Beijing, China), and the Caspase-2 cellular activity assay kit was purchased from the Nanjing Jiancheng Bioengineering Institute (Nanjing, China). The LDH Activity Assay Kit was purchased from Abcam. The miR-34a mimic oligonucleotide and control RNA were purchased from GenePharma (Shanghai, China). The Lipofectamine™ 2000 reagent was obtained from Invitrogen Life Technologies (Carlsbad, CA, USA). Antibodies for the Western blot assay were purchased as follows: XBP1, IRE1α, and p-IRE1α antibodies (Abcam, Cambridge, UK) and Caspase-2 and β-actin antibodies (Sigma-Aldrich, St. Louis, MO, USA). All culture media and fetal bovine serum (FBS) were obtained from Gibco (Carlsbad, CA, USA). Unless specifically mentioned, all other reagents were purchased from Sigma-Aldrich.

2.2. Aβ Peptide Preparation

Aβ1-40 was dissolved in double deionized water at a concentration of 200 μmol/l and was stored at −80°C. To increase the toxicity, it was incubated at 37°C for 24 h before use in each of the experiments according to our previous study [24], after which it was diluted to the required concentration.

2.3. Cell Culture and Treatment

Human neuroblastoma SH-SY5Y cells were purchased from the Institute of Basic Medical Sciences of the Chinese Academy of Medical Sciences and were cultured in RPMI 1640 medium supplemented with 10% FBS, 300 μg/ml glutamine, 100 μg/ml streptomycin, and 100 U/ml penicillin. Cells were maintained at 37°C in an incubator containing 5% CO₂. When grown to 90% confluence, cells were washed with serum-free medium and then treated with various concentrations of Aβ1-40 (0, 1, 3, or 5 μM) for 0–48 h. In the inhibition studies, cells were pretreated with STF-083010 (10, 30, 60, or 100 μM) for 6 h, followed by exposure to 5 μM Aβ1-40 for another 24 h [25]. Cell morphology was observed with a phase contrast microscope (AE31; Motic, China).

2.4. Transfection

SH-SY5Y cells () were seeded into 6-well plates and cultured for 24 h. On the following day, cells were transfected with 100 nM of miR-34a mimic oligonucleotide or a nonspecific control RNA using the Lipofectamine™ 2000 reagent, according to the manufacturer’s instructions. The following sequences were used: miR-34a mimic oligonucleotide 5-UGGCAGUGUCUUAGCUGGUUGU-3 and negative control 5-UCCUAACCGCGUGUCACGUTT-3. Specifically, serum-free MEM medium (250 μl) was used to dilute the miR-34a mimic (10 μl) and NC. Then, 5 μl of Lipofectamine 2000 was diluted with 250 μl of the same medium and incubated at room temperature for 5 min. The diluted miR-34a mimic or NC was then mixed with the diluted Lipofectamine 2000 and incubated for 20 min at room temperature to allow for complex formation. The complexes were then added to each well containing the SH-SY5Y cells and placed in a 37°C/5% CO₂ incubator. After 6 h, the cultures were replaced with 2 ml fresh medium supplemented with 10% FBS. Forty-eight hours after transfection, cells were incubated using 5 μM Aβ1-40 for 24 h.

2.5. Cytotoxicity Assessment

The viability of SH-SY5Y cells was measured by the 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT) assay. SH-SY5Y cells were seeded into 96-well plates at a density of cells per well and cultured at 37°C in culture medium for 24 h. Cells were washed in sodium medium, 20 μl MTT (5 mg/ml) was added to the cells, and they were cultured at 37°C for 4 h before the addition of stop solution, which was added to dissolve MTT. The absorbance of samples was measured at 490 nm with a microplate reader. Data are presented as the percentage of survival relative to normal cultured cells without any treatment.

The integrity of the plasma membrane was evaluated by determining the release of the cytoplasmic enzyme LDH. The cells were subjected to different treatments. Subsequently, the activity of released LDH was examined according to the instructions of the LDH Activity Assay Kit. Absorbance was measured at a wavelength of 490 nm. The LDH release was expressed as a percentage relative to the positive control group.

2.6. Western Blot Assay

After drug treatment, SH-SY5Y cells were harvested and total protein was isolated. The protein concentration was determined by BCA assay. Equal amounts of protein were resolved in 10% SDS-PAGE followed by transfer to a nitrocellulose membrane. Membranes were blocked with 5% fat-free milk in TBST and then immunoblotted with an anti-p-IRE1α antibody (diluted 1 : 1000), anti-IRE1α antibody (diluted 1 : 1000), anti-XBP1 antibody (diluted 1 : 1000), anti-Caspase-2 antibody (diluted 1 : 1000), or anti-actin antibody (diluted 1 : 1000) at room temperature for 1.5 h. Membranes were washed and incubated with peroxidase-conjugated secondary antibodies at room temperature for 1 h. Subsequently, membranes were exposed to chemiluminescence reagents. Protein expression was quantified using the AlphaEase FC image analysis software.

2.7. Reverse Transcription Polymerase Chain Reaction (RT-PCR)

Reverse transcription-PCR was performed to examine the expression of spliced-XBP1 mRNA. Briefly, the total RNA was extracted using the RNApure Total RNA Fast Isolation Kit. Equal amounts of RNA were used for reverse transcription with M-MLV reverse transcriptase, according to the manufacturer’s instructions. The cDNAs were then used for PCR amplification. The primers used are listed in Table 1. The following PCR program was used: 95°C for 5 min, followed by 36 cycles of 20 sec at 95°C, 20 sec at 52°C, and 30 sec at 72°C. β-Actin served as the internal control for data normalization. PCR products were separated on acrylamide gels containing 7.5% acrylamide for XBP1 PCR products. For quantitative analysis, intensities of DNA bands were quantified using software.

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

The expression level of miR-34a was determined by qRT-PCR. Briefly, total RNA was isolated from cells using the RNApure Total RNA Fast Isolation Kit and was then reverse-transcribed using the Power RT Kit. Real-time PCR was performed using 2x Power Taq PCR MasterMix and SYBR Green on a Superior 5-color Real-Time Quantitative PCR system (Bioneer, Korea). The primers for mature miR-34a and U6 were purchased from Sangon Biotech (China). The primers used are listed in Table 2. The relative amount of miR-34a was normalized to the U6 snRNA, and the fold change in each miRNA was calculated using the 2^-ΔΔCt method [26].

2.9. Measurement of Caspase-2 Activity in SH-SY5Y Cells

Caspase-2 activity was measured in the lysates of SH-SY5Y cells using the Caspase-2 cellular activity assay kit. Briefly, SH-SY5Y cells were cultured as described above. After washing and trypsinization, cell suspensions were centrifuged (400 g, 3 min, 4°C), and cell pellets were resuspended in 100 μl of ice-cold cell lysis buffer and incubated for 15 min. Following centrifugation (16,000 g, 15 min, 4°C), supernatants were collected, and enzyme activity was measured according to the manufacturer’s instructions. The reaction mixtures (total volume 100 μl) were incubated at 37°C overnight, and the optical density value was measured at 405 nm using a microplate reader.

2.10. Statistical Analysis

Data are presented as (SEM). Each procedure was performed in four independent experiments. Statistical analyses were performed using a one-way analysis of variance (ANOVA), followed by an LSD post hoc test. A value < 0.05 was considered significant. All statistical analyses were performed using SPSS software version 13.0.

3. Results

3.1. Aβ1-40 Induced Cytotoxicity of SH-SY5Y Cells

We examined the effect of Aβ on the cytotoxicity of SH-SY5Y cells by MTT and LDH assay. Aβ1-40 induced a concentration- and duration-dependent decrease in the viability of SH-SY5Y cells. Exposure to 1, 3, or 5 μM of Aβ1-40 reduced the survival of SH-SY5Y cells to , , and of the control, respectively (Figure 1(a), ). We used LDH to further determine the cell viability. Similar to that observed in the MTT assay, Aβ1-40 treatment increased LDH release from to , , and (Figure 1(c), ). Exposure to 5 μM Aβ1-40 resulted in sufficient toxicity in the cells and was used in subsequent studies. Exposure to 5 μM of Aβ1-40 for 6, 12, 24, or 48 h reduced the survival of SH-SY5Y cells to , , , and of that of the control, respectively (Figure 1(b), ). Exposure to 5 μM of Aβ1-40 for 6, 12, 24, or 48 h increased the LDH release to , , , or , respectively (Figure 1(d), ).

(a)

(b)

(c)

(d)

3.2. Activation of the IRE1 Signaling Pathway in Aβ-Treated SH-SY5Y Cells

The IRE1 signaling pathway through XBP1 is strongly linked with ER stress and UPR. To investigate whether IRE1α-mediated UPR post-Aβ1-40 injury is activated, spliced-XBP1 mRNA was measured by RT-PCR. The expression of IRE1α, phosphorylated IRE1α (p-IRE1α), and XBP1s in SH-SY5Y cells was measured by Western blotting. Exposure to Aβ1-40 (5 μM) for 24 h increased the level of the spliced-XBP1 mRNA in SH-SY5Y cells (2.29-fold vs. control, ) (Figures 2(a) and 2(b)). Increased expression of the p-IRE1α (1.61-fold vs. control, ) (Figures 2(c) and 2(d)) and spliced-XBP1 (XBP1s) proteins was also observed in Aβ-treated SH-SY5Y cells (1.80-fold vs. control, ) (Figures 2(c) and 2(d)). STF-083010, an inhibitor of IRE1’s RNase, was applied to prevent the splicing of XBP1. We found that STF-083010 inhibits IRE1α in a dose-dependent manner and the effect was reflected by XBP1 splicing. XBP1 splicing was reduced to normal levels when treated with STF-083010 at 60 μM or above (, Figures 2(c) and 2(d)). Total IRE1α remained unchanged post-Aβ1-40 injury and STF-081030 treatment. At the same time, STF-081030 treatment could not alleviate the overexpression of p-IRE1α after Aβ1-40 injury. These results suggest that STF-083010 blocks IRE1-dependent splicing of XBP1 but not IRE1-autophosphorylation in response to Aβ (1-40) (Figures 2(c) and 2(d)).

(a)

(b)

(c)

(d)

Figure 2

Activation of the IRE1 signaling pathway in Aβ-treated SH-SY5Y cells. SH-SY5Y cells were incubated with 5 μM Aβ1-40 for 24 h. The spliced-XBP1 level was detected by RT-PCR. (a) Representative RT-PCR data showing the spliced-XBP1 bands. (b) Densitometric analysis of the spliced-XBP1 level normalized to the β-actin level. The cultured SH-SY5Y cells were pretreated with STF-083010 (0, 10, 30, 60, or 100 μM) for 6 h, followed by exposure to 5 μM Aβ1-40 under the continued presence of STF-083010 for 24 h. The levels of XBP1s, p-IRE1α, and IRE1α were detected by Western blotting. (c) Representative Western blot showing the XBP1s, p-IRE1α, and IRE1α bands. (d) Densitometric analysis of the protein levels of XBP1s, p-IRE1α, and IRE1α normalized to the β-actin level. The values are presented as the from four independent experiments. compared with the control. ^# compared with the Aβ1-40-alone group. ^## compared with the Aβ1-40-alone group.

3.3. IRE1α Inhibition Upregulated miR-34a Expression

To explore the mechanistic bases of IRE1α-mediated Aβ1-40 injury, we turned our attention to miR-34a, a candidate target of IRE1α’s endonuclease activity. SH-SY5Y cells were exposed to Aβ1-40 (5 μM) for 0, 2, 6, or 24 h. Quantitative real-time PCR was used to determine the miR-34a levels in different groups. The level of miR-34a was increased after treatment with Aβ1-40 (5 μM) for 2 h and 6 h, which peaked at 2 h and then started to decrease. At 24 h, the miR-34a levels had decreased to 84.0% of the control (Figure 3, ). To confirm that IRE1α acts as a negative regulator of miR-34a under Aβ1-40 conditions, we examined the miR-34a levels after IRE1α inhibition. As shown in Figure 4(a), STF-083010 partially prevented the Aβ-induced decrease in miR-34a levels (97.0% of control levels, ). Treatment with 60 μM STF-083010 alone had no effect on miR-34a levels, with no significant difference compared with the control group.

(a)

(b)

(c)

(d)

(e)

(f)

Figure 4

The roles of IRE1α and miR-34a in Aβ-induced toxicity in SH-SY5Y cells. Cells were incubated with STF-083010 (60 μM)+Aβ1-40 (5 μM), STF-083010 (60 μM) alone, or Aβ1-40 (5 μM) alone or were untreated. In transfection studies, cells were transfected with the miR-34a mimic oligonucleotide or nonspecific control in the presence or absence of Aβ1-40 (5 μM). (a) miR-34a levels were measured using quantitative real-time PCR. (b) Cell viability was measured using the MTT assay. (c) The integrity of the plasma membrane was assessed by LDH release. (d) Caspase-2 activity was measured using the Caspase-2 cellular activity assay kit. (e) The expression of Caspase-2 was measured by Western blotting. (f) Morphological analysis of SH-SY5Y cells by microscopy. Scale bar: 100 mm. Data are presented as the from four independent experiments. compared with the control; ^## compared with the Aβ1-40-alone group.

3.4. Both IRE1α Inhibition and miR-34a Transfection Reduce Aβ Neurotoxicity

To determine whether IRE1α contributes to the Aβ-induced death of SH-SY5Y cells, we inhibited IRE1α using a specific inhibitor of IRE1α. As illustrated in Figure 4(b), Aβ1-40 (5 μM for 24 h) treatment decreased cell viability to . Pretreatment with STF-083010 (60 μM) significantly mitigated the Aβ1-40-induced death of SH-SY5Y cells, restoring cell viability to (). STF-083010 at 60 μM alone did not cause any apparent cytotoxicity. This result was confirmed by LDH analysis, which showed that STF-083010 alleviated Aβ-induced cytotoxicity in SH-SY5Y cells. Aβ1-40 treatment increased LDH release from to . Pretreatment with STF-083010 (60 μM) restored LDH release to . Taken together, these data indicate that IRE1α are indeed involved in Aβ-induced neurotoxicity.

We also examined cell viability in SH-SY5Y cells transfected with the miR-34a mimic oligonucleotide or a nonspecific control to determine whether miR-34a regulates cell viability in Aβ1-40-treated SH-SY5Y cells. miR-34a levels were markedly increased in SH-SY5Y cells transfected with the miRNA-34a mimic oligonucleotide (1.21-fold vs. control, , Figure 4(a)), with no change observed in SH-SY5Y cells transfected with the control oligonucleotide. As shown in Figure 4(b), the miRNA-34a mimic oligonucleotide restored cell viability to (), significantly higher than the Aβ-alone group. The cell viability in SH-SY5Y cells transfected with control oligonucleotide showed no significant changes. This result was confirmed by LDH analysis, which showed that in SH-SY5Y cells transfected with the miR-34a mimic oligonucleotide, Aβ-induced cytotoxicity was alleviated, restoring LDH release to (, Figure 4(c)).

3.5. Both IRE1α Inhibition and miR-34a Transfection Reduce the Activation of Caspase-2

We investigated Caspase-2 expression and activity after exposure to Aβ1-40 and STF-083010, as described above, to evaluate the role of IRE1α in Aβ-induced activation of Caspase-2 in SH-SY5Y cells. As illustrated in Figure 4(d), Caspase-2 activity was significantly increased by Aβ1-40 (2.10-fold vs. control; ), which was partially prevented by STF-083010 (1.46-fold vs. control, ). Treatment with 60 μM STF-083010 alone had no effect on Caspase-2 activity. Western blotting demonstrated that Aβ resulted in an increase in the Caspase-2 protein expression (4.04-fold vs. control, ), while Caspase-2 levels were markedly decreased in SH-SY5Y cells pretreated with STF-083010 (60 μM) for 6 h (33.53% of the Aβ-alone group, Figure 4(e), ).

We also examined the Caspase-2 expression and activity in SH-SY5Y cells transfected with the miR-34a mimic oligonucleotide or a nonspecific control to determine whether miR-34a regulates Caspase-2 activation in Aβ1-40-treated SH-SY5Y cells. As illustrated in Figure 4(d), after miR-34a mimic transfection, Caspase-2 activity was markedly decreased (54.58% of the Aβ-alone group, ). Caspase-2 activity in SH-SY5Y cells transfected with control oligonucleotide showed no significant changes. Caspase-2 levels were markedly decreased in SH-SY5Y cells transfected with the miR-34a mimic oligonucleotide (31.2% of the Aβ-alone group, ). The expression levels of Caspase-2 in SH-SY5Y cells transfected with control oligonucleotide showed no significant changes (Figure 4(e)).

3.6. Morphology of SH-SY5Y Cells

SH-SY5Y cells were treated according to the protocol described in Materials and Methods. As shown in Figure 4(f), visible morphological changes were observed during the treatment in cells. SH-SY5Y in the normal group adhered to the wall after 24 h of inoculation. The majority of the cells were oval and triangular in shape. The nucleus was easy to distinguish from the perikaryon. Most of the cells grew more than 2 protrusions, and most of the protrusions came into contact with adjacent cells or protrusions. However, when exposed to Aβ1-40 (5 μM) for 24 h, most of the cells showed significant morphological changes, such as loss of neurites, detaching from the surface, forming clusters, and having an irregular cell shape. The number of cells injured and the degree of cell injury were significantly improved when the cells were pretreated with 60 μM STF-083010 or transfected with the miR-34a mimic oligonucleotide, while STF-083010 treatment alone did not show morphological alterations, and transfection with nonspecific control oligonucleotide had no effect on improving the cell injury.

4. Discussion

The Aβ peptide has been reported to cause apoptosis by activating ER stress-specific caspases [5, 27]. However, induction of the IRE1 signaling pathway by Aβ was not shown in these studies. As an RNase, IRE1α targets and regulates the expression of a number of RNAs (both coding and noncoding) [22, 23]. As a downstream target of IRE1α, XBP1 is one of the most well-studied genes modulated by IRE1α and plays important roles in regulating cell survival and the UPR [13]. A previous study has reported that AD progression at the histopathological level is associated with chronic IRE1 activation in the brain and IRE1 deficiency significantly reduces the accumulation of Aβ in the brain of 5xFAD mice [28]. In this study, we uncovered the other role of IRE1 in the pathogenesis of AD. We investigated the effects of Aβ1-40 on activation of the IRE1 signaling pathway by determining the levels of the phosphorylated form of IRE1α and spliced XBP1. Aβ significantly increased the levels of the p-IRE1α protein and the spliced XBP1, revealing that the IRE1 signaling pathway was activated in Aβ-treated cells. The Aβ peptide induces Ca²⁺ release from the ER, potentially resulting in Ca²⁺ depletion in the ER lumen. The depletion of ER Ca²⁺ disturbs the posttranslation modification and folding of proteins, leading to the accumulation of unfolded and misfolded proteins in the ER lumen and subsequent induction of ER stress [29, 30]. The evidence provided in our study will be helpful in improving our understanding of the mechanism by which the Aβ peptide induces ER stress. The activation of the IRE1 signal pathway observed in this study may be associated with abnormal Ca²⁺ signaling.

According to recent studies, miR-34a is cleaved by IRE1α, resulting in activation of Caspase-2 in mouse embryonic fibroblasts (MEFs) [22, 23]. We examined the levels of miR-34a in SH-SY5Y cells treated with Aβ1-40 and STF-081030, which displays IRE1α RNase inhibitory activity [31], to assess whether the cleavage of miR-34a also occurs in SH-SY5Y cells treated with Aβ1-40 and investigate whether IRE1α is involved in this process. Our results show that IRE1 activation downregulated miR-34a expression. In previous studies, miR-34a was overexpressed in specific brain regions of patients with AD, as well as in the 3xTg-AD mouse model. However, in our study, we observed a dynamic change in miR-34a expression in Aβ1-40-treated SH-SY5Y cells. Increases and decreases in the miR-34a level were detected at different times after Aβ treatment. The discrepancies between the results from these studies and our findings indicate that the mechanism modulating the miR-34a expression differs between cell culture models and neurodegenerative conditions and another pathological process may be involved in the abnormal expression of miR-34a in the brains of patients with AD. Further studies in relevant experimental models are warranted. The present study provides the first description of miR-34a expression in response to Aβ-induced ERS, which may lead to the discovery of new mechanisms.

Based on the results from the present study, exposure to Aβ clearly resulted in a decrease in cell viability, and cell death was mediated by a caspase-dependent mechanism. Caspase-2, a member of the cysteine protease family, is one of the targets of miR-34a [22]. Our study provides evidence that downregulation of the miR-34a expression in Aβ1-40-treated SH-SY5Y cells may increase Caspase-2 activity and potentially contribute to apoptotic cell death. Additionally, an IRE1α inhibitor aided in preventing the effect of Aβ1-40 on miR-34a levels and Caspase-2 activity. Thus, both IRE1α and miR-34a are involved in Aβ-induced cytotoxicity, and this effect may be mediated by Caspase-2, a well-characterized regulator of apoptosis. Transfection of the miR-34a mimic, which protects miR-34a from degradation by IRE1, decreased the levels of the Caspase-2 protein, as shown in the Western blots. Further investigations are required to determine how Caspase-2 and its downstream targets contribute to these cellular processes during ER stress. The IRE1α inhibitor may have the potential to divert apoptosis in response to ER stress by modulating the miR-34a level. These results were further confirmed by morphological observation. However, we cannot conclude that miR-34a is the only microRNA involved in Aβ1-40-induced cytotoxicity, and additional analyses are necessary to explore the levels of microRNAs in clinical specimens. In addition, an examination of the protein and mRNA levels of the other known targets of miR-34a is necessary to determine whether these proteins are also involved in this process.

5. Conclusion

Taken together, our findings identify a previously unrecognized mechanism by which the Aβ peptide regulates Caspase-2 expression and activity to induce cytotoxicity that involves both IRE1α and a noncoding RNA (miR-34a). Our study may prompt the development of a novel therapeutic strategy that targets IRE1α and miR-34a to treat AD.

Data Availability

The data used to support the findings of this study are available from the corresponding author upon request.

Conflicts of Interest

The authors declared no conflict of interest.

Acknowledgments

This research was supported by the Harbin Medical University Scientific Research Innovation Fund (No: 2016lczx45) and China Postdoctoral Science Foundation (No: 2017M611387).

References

O. Almkvist, “Functional brain imaging as a looking-glass into the degraded brain: reviewing evidence from Alzheimer disease in relation to normal aging,” Acta Psychologica, vol. 105, no. 2-3, pp. 255–277, 2000.
View at: Publisher Site | Google Scholar
W. Annaert and B. De Strooper, “A cell biological perspective on Alzheimer’s disease,” Annual Review of Cell and Developmental Biology, vol. 18, no. 1, pp. 25–51, 2002.
View at: Publisher Site | Google Scholar
D. J. Selkoe, “Cell biology of protein misfolding: the examples of Alzheimer’s and Parkinson’s diseases,” Nature Cell Biology, vol. 6, no. 11, pp. 1054–1061, 2004.
View at: Publisher Site | Google Scholar
J. P. Taylor, J. Hardy, and K. H. Fischbeck, “Toxic proteins in neurodegenerative disease,” Science, vol. 296, no. 5575, pp. 1991–1995, 2002.
View at: Publisher Site | Google Scholar
T. Nakagawa, H. Zhu, N. Morishima et al., “Caspase-12 mediates endoplasmic-reticulum-specific apoptosis and cytotoxicity by amyloid-beta,” Nature, vol. 403, no. 6765, pp. 98–103, 2000.
View at: Publisher Site | Google Scholar
M. Boyce and J. Yuan, “Cellular response to endoplasmic reticulum stress: a matter of life or death,” Cell Death and Differentiation, vol. 13, no. 3, pp. 363–373, 2006.
View at: Publisher Site | Google Scholar
W. Paschen and T. Mengesdorf, “Endoplasmic reticulum stress response and neurodegeneration,” Cell Calcium, vol. 38, no. 3-4, pp. 409–415, 2005.
View at: Publisher Site | Google Scholar
Y. Chen and F. Brandizzi, “IRE1: ER stress sensor and cell fate executor,” Trends in Cell Biology, vol. 23, no. 11, pp. 547–555, 2013.
View at: Publisher Site | Google Scholar
D. Han, A. G. Lerner, L. Vande Walle et al., “IRE1α kinase activation modes control alternate endoribonuclease outputs to determine divergent cell fates,” Cell, vol. 138, no. 3, pp. 562–575, 2009.
View at: Publisher Site | Google Scholar
N. Plongthongkum, N. Kullawong, S. Panyim, and W. Tirasophon, “Ire1 regulated XBP1 mRNA splicing is essential for the unfolded protein response (UPR) in Drosophila melanogaster,” Biochemical and Biophysical Research Communications, vol. 354, no. 3, pp. 789–794, 2007.
View at: Publisher Site | Google Scholar
A. B. Tam, A. C. Koong, and M. Niwa, “Ire1 has distinct catalytic mechanisms for XBP1/HAC1 splicing and RIDD,” Cell Reports, vol. 9, no. 3, pp. 850–858, 2014.
View at: Publisher Site | Google Scholar
A. Uemura, M. Oku, K. Mori, and H. Yoshida, “Unconventional splicing of XBP1 mRNA occurs in the cytoplasm during the mammalian unfolded protein response,” Journal of Cell Science, vol. 122, Part 16, pp. 2877–2886, 2009.
View at: Publisher Site | Google Scholar
R. Wu, Q. H. Zhang, Y. J. Lu, K. Ren, and G. H. Yi, “Involvement of the IRE1α-XBP1 pathway and XBP1s-dependent transcriptional reprogramming in metabolic diseases,” DNA and Cell Biology, vol. 34, no. 1, pp. 6–18, 2015.
View at: Publisher Site | Google Scholar
C. Hetz, F. Martinon, D. Rodriguez, and L. H. Glimcher, “The unfolded protein response: integrating stress signals through the stress sensor IRE1α,” Physiological Reviews, vol. 91, no. 4, pp. 1219–1243, 2011.
View at: Publisher Site | Google Scholar
J. Hollien and J. S. Weissman, “Decay of endoplasmic reticulum-localized mRNAs during the unfolded protein response,” Science, vol. 313, no. 5783, pp. 104–107, 2017.
View at: Publisher Site | Google Scholar
E. Sonkoly and A. Pivarcsi, “MicroRNAs in inflammation,” International Reviews of Immunology, vol. 28, no. 6, pp. 535–561, 2009.
View at: Publisher Site | Google Scholar
E. van Rooij and E. N. Olson, “MicroRNA therapeutics for cardiovascular disease: opportunities and obstacles,” Nature reviews Drug Discovery, vol. 11, no. 11, pp. 860–872, 2012.
View at: Publisher Site | Google Scholar
S. Lin and R. I. Gregory, “MicroRNA biogenesis pathways in cancer,” Nature Reviews Cancer, vol. 15, no. 6, pp. 321–333, 2015.
View at: Publisher Site | Google Scholar
M. Y. Wong, Y. Yu, W. R. Walsh, and J. L. Yang, “MicroRNA-34 family and treatment of cancers with mutant or wild-type p53 (review),” International Journal of Oncology, vol. 38, no. 5, pp. 1189–1195, 2011.
View at: Publisher Site | Google Scholar
Y. T. Qi, Y. Zhao, Z. Zhang et al., “The expression pattern and possible function of microRNA-34a in neurons,” Journal of Molecular Cell Biology, vol. 42, no. 3-4, pp. 217–223, 2009.
View at: Google Scholar
X. Wang, P. Liu, H. Zhu et al., “miR-34a, a microRNA up-regulated in a double transgenic mouse model of Alzheimer’s disease, inhibits bcl2 translation,” Brain Research Bulletin, vol. 80, no. 4-5, pp. 268–273, 2009.
View at: Publisher Site | Google Scholar
J.-P. Upton, L. Wang, D. Han et al., “IRE1α cleaves select microRNAs during ER stress to derepress translation of proapoptotic caspase-2,” Science, vol. 338, no. 6108, pp. 818–822, 2012.
View at: Publisher Site | Google Scholar
J. Hassler, S. S. Cao, and R. J. Kaufman, “IRE1, a double-edged sword in pre-miRNA slicing and cell death,” Developmental Cell, vol. 23, no. 5, pp. 921–923, 2012.
View at: Publisher Site | Google Scholar
Q. Li, J. Fang, M. Yang, D. Wu, L. Zhang, and Y. Zhang, “Galantamine inhibits calpain-calcineurin signaling activated by beta-amyloid in human neuroblastoma SH-SY5Y cells,” Neuroscience Letters, vol. 480, no. 3, pp. 173–177, 2010.
View at: Publisher Site | Google Scholar
I. Papandreou, N. C. Denko, M. Olson et al., “Identification of an IRE1α endonuclease specific inhibitor with cytotoxic activity against human multiple myeloma,” Blood, vol. 117, no. 4, pp. 1311–1314, 2011.
View at: Publisher Site | Google Scholar
K. J. Livak and T. D. Schmittgen, “Analysis of relative gene expression data using real-time quantitative PCR and the 2^−ΔΔC_T method,” Methods, vol. 25, no. 4, pp. 402–408, 2001.
View at: Publisher Site | Google Scholar
J. Hitomi, T. Katayama, Y. Eguchi et al., “Involvement of caspase-4 in endoplasmic reticulum stress-induced apoptosis and Aβ-induced cell death,” The Journal of Cell Biology, vol. 165, no. 3, pp. 347–356, 2004.
View at: Publisher Site | Google Scholar
C. Duran-Aniotz, V. H. Cornejo, S. Espinoza et al., “IRE1 signaling exacerbates Alzheimer’s disease pathogenesis,” Acta Neuropathologica, vol. 134, no. 3, pp. 489–506, 2017.
View at: Publisher Site | Google Scholar
M. P. Mattson, F. M. LaFerla, S. L. Chan, M. A. Leissring, P. N. Shepel, and J. D. Geiger, “Calcium signaling in the ER: its role in neuronal plasticity and neurodegenerative disorders,” Trends in Neurosciences, vol. 23, no. 5, pp. 222–229, 2000.
View at: Publisher Site | Google Scholar
W. Paschen, “Role of calcium in neuronal cell injury: which subcellular compartment is involved?” Brain Research Bulletin, vol. 53, no. 4, pp. 409–413, 2000.
View at: Publisher Site | Google Scholar
C. L. Kriss, J. A. Pinilla-Ibarz, A. W. Mailloux et al., “Overexpression of TCL1 activates the endoplasmic reticulum stress response: a novel mechanism of leukemic progression in mice,” Blood, vol. 120, no. 5, pp. 1027–1038, 2012.
View at: Publisher Site | Google Scholar

Copyright

Copyright © 2019 Qianqian Li 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.

PDF Download Citation

Download other formats

Order printed copies

Views

1090

Downloads

826

Citations