Apoptosis is considered a crucial part of the host defense system in oysters according to previous reports; however, the exact process by which this occurs remains unclear. Besides, mitochondrial apoptosis is the primary method of apoptosis in vertebrate cells, but has been poorly studied in invertebrates and is quite controversial. In this study, we investigated the molecular mechanism of mitochondrial apoptosis in the Pacific oyster Crassostrea gigas. Notably, we show that most key elements involved in the vertebrate mitochondrial apoptosis pathway – including mitochondrial outer membrane permeabilization, cytochrome c release, and caspase activation – are also present in C. gigas. In contrast, the lack of Bcl-2 homology 3-only subfamily members and apoptotic protease activating factor-1 (APAF-1) protein revealed evolutionary diversity from other phyla. Our results support that mitochondrial apoptosis in animals predates the emergence of vertebrates, but suggest that an unexpectedly diverse mitochondrial apoptosis pathway may exist in invertebrates. In addition, our work provided new clues for an improved understanding of how bivalve acclimate themselves to an inconstant environment.
Oysters live in estuarine and intertidal zones and are constantly exposed to fluctuating temperatures, variable salinity, toxic metals, and desiccation because of their sessile behavior.1 Apoptosis is involved in the response to various stressors and an important host defense mechanism in oysters. For instance, apoptosis participates in the oyster’s defense to Perkinsus marinus, an intracellular protozoan that can cause lethal infection.2 Others have also shown that exposure to cadmium and copper elevates apoptosis levels in oysters.3, 4 The recent application of high-throughput sequencing in marine biology studies has revealed the extensive involvement of apoptosis-related genes in various stress responses, including those to virus,5 air exposure,1 hyperthermia,6 and low salinity.7 However, no studies have focused on elucidating the molecular pathways regulating apoptosis in oyster and the exact physiological mechanisms remain vague, hindering our understanding of how this sedentary animal adapts to its fickle environment.
The mitochondrial or intrinsic apoptosis pathway is characterized by the participation of mitochondria in apoptotic signaling and has been extensively described in vertebrates, including mammals8, 9 and amphibians.10, 11 Several genes homologous to mammalian apoptosis effectors have been identified in invertebrates in recent years,12, 13, 14, 15 seemingly indicative of the existence of a mitochondrial apoptosis pathway in these species.
In comparison with the breadth of data on the molecular physiology of mammalian mitochondrial apoptosis, relatively few mechanisms in invertebrates have been elucidated.16, 17, 18, 19 Nevertheless, current evidence suggests an increased diversity of pathway effectors in these species. For instance, mitochondrial outer membrane permeabilization (MOMP) and cytochrome c release – hallmarks of vertebrate mitochondrial apoptosis – had no role in mitochondrial apoptosis in the nematode Caenorhabditis elegans.16 More specifically, cell death protein 4 – the C. elegans apoptotic protease activating factor-1 (APAF-1) homolog – lacks the WD domain responsible for its interaction with cytochrome c.16 Similarly, although the Drosophila APAF-1-related killer (ARK) homolog contains this region,17 no biochemical evidence exists on the involvement of cytochrome c in ARK activation and induction of the apoptosis cascade.20 As such, additional work is needed to determine the extent of this diversity in invertebrate mitochondrial apoptosis and further understand the pathway’s evolution in animals.
Cursory studies on bivalve apoptosis have been performed,21, 22, 23, 24, 25 yet the exact mechanism of mitochondrial apoptosis remains unclear. This study has three specific goals and therefore includes three aspects of work. First, to investigate whether MOMP and cytochrome c are involved in mitochondrial apoptosis of oyster, we tested the mitochondrial membrane potential (MMP) and subcellular distribution of cytochrome c in UV-irradiated oyster hemocytes. Second, to examine whether members of oyster caspase family regulate mitochondrial apoptosis, activities of caspase 9 and caspase 3 in hemocytes and cytosolic extracts of oyster upon distinct treatments were measured. Third, to elucidate the regulatory roles of Bcl-2 family and p53 in mitochondrial apoptosis pathway of oyster, multiple functional assays were performed. Given that oyster cell lines are not widely available currently, mammalian and yeast cells were used in several assays as molecular tools, which is a typical practice for species without established cell lines.18, 19, 26 Our work significantly improves mechanism understanding of mitochondrial apoptosis pathway in the Pacific oyster and expands our knowledge of evolutionary diversity of apoptosis system in invertebrates.
UV irradiation results in loss of MMP and cytochrome c release in Crassostrea gigas
UV irradiation is an effective apoptosis-inducing factor in many species, including bivalves.25, 27, 28, 29 Thus, we irradiated C. gigas hemocytes with UV light and found a markedly higher percentage of apoptotic cells when compared with non-irradiated controls (Figure 1a). In addition, transmission electron microscopy (TEM) analysis showed the presence of apoptotic cells under UV light irradiation (Supplementary Fig S1), further indicating that UV irradiation was an efficacious apoptosis-inducing factor in C. gigas.
The loss of MMP (ΔΨm) is an indication of early stage of apoptosis, as it is associated with MOMP in vertebrates.30 Thus, we examined MMP with JC-1 assays to determine whether mitochondrial apoptosis in Pacific oyster involved an increase in mitochondrial outer membrane permeability. Notably, irradiated hemocytes exhibited a significant decrease in MMP at 6 h post irradiation (hpi), which further decreased at 9 hpi and 24 hpi (Figure 1b), indicating the existence of an MOMP-like process in UV irradiation-induced apoptosis in C. gigas.
Vertebrate MOMP results in cytochrome c release and triggers mitochondria-mediated apoptosis. To determine whether cytochrome c release occurred in C. gigas cells, UV-irradiated hemocytes were subjected to cytosolic/mitochondrial subcellular fractionation at 24 hpi and the presence of cytochrome c was assessed in each fraction. Western blot analysis revealed that cytochrome c was found in the cytosolic protein fraction of irradiated cells, but undetectable in that of untreated cells (Figure 1c), suggesting that UV irradiation induced release of cytochrome c from mitochondria to the cytosol.
Cytochrome c activates caspase 9 and caspase 3 activity
We tested the activities of effector caspase 9 and executioner caspase 3 in oyster hemocytes following UV irradiation and found remarkable elevations in the activity levels of both caspases at 20 hpi (Figures 2a and b), indicating the involvement of C. gigas (Cg)-caspase 9 and Cg-caspase 3 in irradiation-induced apoptosis. We then incubated cytosolic extracts with cytochrome c purified from equine hearts or C. gigas (Cg-Cyt c). Notably, both Cg-caspase 9 and Cg-caspase 3 activity was significantly increased in the presence of cytochrome c from either source (Figures 2c and d). Further, the addition of exogenous deoxyadenosine triphosphate (dATP) enhanced the cytochrome c-mediated-activation of both caspases (Figures 2c and d).
To determine whether Cg-caspase 3 activity was dependent on that of Cg-caspase 9, oyster cytosolic extracts were pretreated with the caspase 9 inhibitor Z-LEHD-FMK before the addition of Cg-Cyt c. As expected, Cg-caspase 9 activity was substantially decreased significantly with the addition of Z-LEHD-FMK (Figure 2c). Moreover, irradiated hemocytes pretreated with Z-LEHD-FMK showed a markedly lower activity for both Cg-caspase 3 and Cg-caspase 9 (Figure 2e), demonstrating that the functions of these caspases in C. gigas were comparable to their vertebrate counterparts.
Identification and expression analysis of Bcl-2 relatives in the Pacific oyster
B-cell lymphoma (Bcl)-2 protein family members are known regulators of mitochondrial apoptosis. We identified seven candidate Bcl-2 homologs in the Pacific oyster by querying the annotated genome database, but none belonged to the pro-apoptotic 'BH3-only' subfamily. Nevertheless, we performed rapid-amplification of cDNA ends or PCR to amplify the entire coding sequence and subsequently validated their genetic sequences.
To study the functional significance of oyster Bcl-2 family members, we selected four candidate genes out of the seven, as they were more closely related to human Bcl-2 family members with regard to the domain architecture. We designated them as Cg-Bcl-2, Cg-Bcl-xl, Cg-Bak, and Cg-Bax based on their homology to human relatives. All of the four candidates contained BH1, BH2, and BH3 domains, whereas only Cg-Bcl-2 had a BH4 domain (Figure 3a). In addition, Cg-Bak and Cg-Bax harbored a transmembrane domain absent in Cg-Bcl-2 and Cg-Bcl-xl (Figure 3a). An amino-acid sequence-based phylogenetic analysis showed that Cg-Bcl-2 and Cg-Bcl-xl clustered into the anti-apoptotic protein category, whereas Cg-Bak and Cg-Bax classified as pro-apoptotic proteins (Figure 3b).
Quantitative PCR (qPCR) analysis was performed to investigate the expression pattern of oyster Bcl-2 family genes in different tissues and under various environmental stresses. All the four genes displayed relatively high expression in gill and hemolymph (Supplementary Figure S2). Moreover, infection with ostreid herpesvirus 1 (OsHV-1, a common virus that can cause mass mortality of oyster) or Vibrio alginolyticus, as well air exposure and heat shock, markedly altered the expressions of these Bcl-2 relatives (Supplementary Figure S3, Supplementary Figure S4,Supplementary Figure S5, and Supplementary Figure S6).
C. gigas Bcl-2 family members regulate apoptosis signaling
We first examined the contributions of the Pacific oyster Bcl-2 candidate homologs in cell death in the yeast Saccharomyces cerevisiae, as Bax and Bak from human31 and Schistosoma mediterranea18 can trigger cell death in yeast according to previous reports. Significantly, we found that both Cg-Bak and Cg-Bax induced yeast cell death (Figure 4a); however, co-expression of either Cg-Bcl-2 or human Bcl-2 rescued yeast from Cg-Bak- or Cg-Bax-induced lethality (Figure 4a).
To further determine the roles of oyster Bcl-2 family members in apoptosis, we overexpressed Cg-Bak or Cg-Bax in HEK293T cells. Interestingly, neither Cg-Bak or Cg-Bax altered caspase 3 activity in these cells, nor did Cg-Bcl-xl or Cg-Bcl-2 (data not shown). However, H2O2-induced oxidative stress effectively stimulated caspase 3 activity level in HEK293T cells, which was markedly increased in counterparts with Cg-Bak or Cg-Bax overexpression (Figures 4b and c). In addition, the co-expression of Cg-Bcl-2 or Cg-Bcl-xl with Cg-Bak or Cg-Bax significantly attenuated the caspase 3 activity in H2O2-treated cells when compared with treated controls with Cg-Bak or Cg-Bax expression alone (Figures 4b and c).
We then analyzed the expression of the four Bcl-2 family genes following UV irradiation and found a remarkable induction of all four candidates (Figure 4d), indicative of their involvement in apoptosis regulation. We performed siRNA assays on Cg-Bak and Cg-Bax, which effectively suppressed their expression (Figures 4e and f). Subsequently, we irradiated Cg-Bak-silenced, Cg-Bax-silenced, and scrambled siRNA-treated hemocytes and measured apoptosis at 3 and 24 hpi, which revealed that Cg-Bak-silenced and Cg-Bax-silenced hemocytes were both significantly more resistant to UV-induced apoptosis than their scrambled siRNA-treated counterparts at 24 hpi (Figures 4g and h).
Cg-Bak and Cg-Bax translocate to the mitochondria and induce cytochrome c release during apoptosis
To understand how the pro-apoptotic oyster Bcl-2 family proteins regulate mitochondrial apoptosis, we studied the subcellular localization of Cg-Bak and Cg-Bax in HeLa cells. Fluorescence microscopy showed that both Cg-Bak and Cg-Bax mainly localized throughout the cytoplasm of normal cells, but translocated to the mitochondria in a subset of cells following UV irradiation. (Figures 5a and b). These data were also validated in subcellular fractionation experiments in HEK293T cells with Cg-Bak and Cg-Bax overexpression (Figure 5c).
To ascertain whether the mitochondrial translocation of Cg-Bak and Cg-Bax was associated with their regulatory roles in apoptosis, we examined the impact of purified Cg-Bak and Cg-Bax protein on isolated oyster mitochondria. When control mitochondria were incubated in storage buffer and centrifuged, cytochrome c could only be detected in the precipitate; however, incubation with CaCl2 resulted in detectable cytochrome c only in the supernatant (Figure 5d). Subsequent analyses showed that cytochrome c was detectable in both the supernatant and precipitate when mitochondria were incubated with recombinant Cg-Bak or Cg-Bax (Figure 5d).
Anti-apoptotic Bcl-2 family proteins directly bind Cg-Bak and Cg-Bax
In mammals, anti-apoptotic Bcl-2 subfamily members interact with their pro-apoptotic counterparts, thereby inhibiting the activities of the latter.32 Thus, we used a yeast two-hybrid system to determine whether this regulatory interaction also occurred with C. gigas homologs. Notably, both Cg-Bcl-2 and Cg-Bcl-xl were found to interact with pro-apoptotic Cg-Bak and Cg-Bax (Figure 6a). A series of truncated mutants were constructed to identify the domain essential for mediating these interactions (Figure 6b). Results of yeast two-hybrid assays with the truncated mutants indicated that the BH3 domain facilitated the interactions between oyster Bcl-2 family members (Figure 6c), which was subsequently confirmed with co-immunoprecipitation (co-IP) assays. (Figures 6d and e).
C. gigas Cg-p53 is involved in mitochondrial apoptosis
Despite the application of high-throughput sequencing technologies, a BH3-only homolog is yet to be discovered in mollusk.21, 33, 34 This absence led us to identify other regulators of mitochondrial apoptosis upstream of the Bcl-2 homologs. We first considered the oyster p53 homolog Cg-p53 as a candidate, as p53 is known to regulate Bcl-2 family activities in mammals.35 Our preliminary analysis of Cg-p53 expression in oyster hemocyte showed a substantial upregulation in response to UV irradiation (Figure 7a). We then treated the hemocytes with the p53 inhibitor pifithrin-α and validated its effect of PFT-α on Cg-p53 expression (Figure 7b). Moreover, analysis of UV irradiation-induced apoptosis in PFT-α-treated hemocytes revealed that p53 inhibition substantially increased their apoptotic resistance at 3 hpi and 6 hpi, but not at 24 hpi, when compared with untreated controls (Figure 7c). This is consistent with an increase of Cg-Bcl-2 and Cg-Bcl-xl levels (Supplementary Figure S7) together with the delay in Cg-Bak activation, thus suggesting that the absence of p53 could promote apoptosis resistance through Cg-Bcl-2 and Cg-Bcl-xl.
Cg-p53 regulates the Bcl-2 family in mitochondrial apoptosis pathway of Pacific oyster
Dual-luciferase reporter assays were used to monitor Cg-p53 transcriptional activity. The ~2 kb region upstream of the Cg-Bak, Cg-Bax, Cg-Bcl-2, and Cg-Bcl-xl start codons were considered as potential promoter regions and used to construct the Cg-Bak-Luc, Cg-Bax-Luc, Cg-Bcl-2-Luc, and Cg-Bcl-xl-Luc plasmids (Figure 8a). In preliminary experiments with HEK293T cells, Cg-p53 elicited the transcription from Cg-Bak-Luc and Cg-Bax-Luc promoters, whereas it repressed the transcription from Cg-Bcl-2-Luc and Cg-Bcl-xl-Luc promoters, all in a dose-dependent manner (Figures 8b–e).
To determine whether Cg-p53 could regulate Cg-Bak and Cg-Bax in oyster cells, the expression patterns of Cg-Bak and Cg-Bax in PFT-α treated hemocytes after UV light irradiation were determined. The qPCR data showed that PFT-α treatment significantly delayed the activation of Cg-Bak expression upon irradiation, compared with that in untreated hemocytes (Figure 8f), indicating that Cg-p53 transactivates Cg-Bak in C. gigas. For Cg-Bax, however, the timing of activation is mostly unchanged in both PFT-α-treated and non-treated hemocytes (Figure 8g).
Considering that mammalian p53 regulates the activities of both anti-apoptotic and pro-apoptotic Bcl-2 family proteins through a transcription-independent way (protein–protein interaction), Cg-p53 may also bind to oyster Bcl-2 family members. This could serve as a plausible explanation for the unexpected absence of Cg-Bax promoter activity in PFT-α treated irradiated hemocytes. Thus, we performed a co-IP assay on Cg-p53 in HEK293T cells with the four Bcl-2 family proteins of C. gigas, yielding positive results; hence, probable interactions exist between the proteins in question (Figure 8h).
The mechanisms of invertebrate mitochondrial apoptosis are unclear. Current evidence demonstrates that neither MOMP and cytochrome c release regulate mitochondrial apoptosis in Drosophila melanogaster and C. elegans; however, these events are essential for that in Schmidtea mediterranea.36, 37, 38, 39 Therefore, further analysis should be carried out in other invertebrate species to elucidate the evolutionary physiology of mitochondrial apoptosis in invertebrates. Herein, we demonstrated the existence of MOMP and cytochrome c release in mitochondrial apoptosis of C. gigas. These results confirmed previous speculation that MOMP and cytochrome c release emerged prior to that of deuterostomes, but somehow missed in ecdysozoa species – at least with respect to Drosophila melanogaster and C. elegans.20
Caspase 9 and caspase 3 are proteases with vital roles in mitochondrial apoptosis. In this study, we found that both Cg-caspase 9 and Cg-caspase 3 were involved in mitochondrial apoptosis in C. gigas, with Cg-caspase 9 likely acting as an upstream activator of Cg-caspase 3 – consistent with their roles in vertebrates.40 However, the oyster APAF-1 homolog lacks the caspase recruitment domain (CARD domain) and only possesses the cytochrome c-interacting WD domain. In fact, no CARD domain-containing APAF-1 homolog has been identified in the Mollusca phylum to date, supporting the existence of a distinct mechanism of caspase 9 activation. Interestingly, the C. elegans APAF-1 homolog contains a CARD domain, but no WD domain,41 indicative of pathway diversity throughout invertebrates.
Bcl-2 family proteins are central regulators of mitochondrial apoptosis. In this study, we identified the existence of oyster Bcl-2 family genes and demonstrated their regulatory roles in apoptosis. Notably, both Cg-Bak and Cg-Bax exhibited pro-apoptotic effects in yeast, consistent with that previously observed with their human31 and S. mediterranea homologs.18 The present work sought to define the functional significance of Cg-Bak and Cg-Bax in mitochondrial apoptosis, and revealed that both factors translocate from the cytoplasm to mitochondria in mammalian cells in response to UV irradiation. This result indicates that while Cg-Bax likely functions in a similar manner to its mammalian counterpart,42, 43 Cg-Bak may utilize an independent mechanisms as mammalian Bak mainly localizes to the mitochondrial outer membrane in healthy cells.44 However, the inconsistencies in Cg-Bak and mammalian Bak subcellular localization might be the result of structural differences or the misfolding of Cg-Bak in mammalian cells. We were unable to examine the distribution of these proteins in oyster cells due to the lack of suitable antibodies. Despite this, the result herein could still imply the association of the proteins with mitochondria during apoptosis. In fact, our previous study demonstrates a potential interaction between Cg-Bak and the mitochondrial outer membrane porin Cg-VDAC2.45 Nevertheless, our results support that Cg-Bak and Cg-Bax induce cytochrome c release, as observed with mammalian Bak and Bax. Moreover, our study also revealed that the interaction of anti-apoptotic proteins (Cg-Bcl-2 and Cg-Bcl-xl) and pro-apoptotic proteins (Cg-Bak and Cg-Bax) in C. gigas was mediated by the BH3 domain, consistent with vertebrates.46, 47 In addition, whereas Cg-Bak was found to be transcriptional activated by Cg-p53, Cg-Bax seemed to be more loosely regulated, although its promoter could be activated by Cg-p53 in mammalian cells. This might not result from the regulation by Cg-Bcl-2 or Cg-Bcl-xl, as the anti-apoptotic Bcl-2 family members were both negatively regulated by Cg-p53. Therefore, it will be an interesting work to clarify the mechanisms regulating Cg-Bax. Collectively, the apoptotic functions of the oyster Bcl-2 family proteins investigated here are fairly conserved with vertebrate counterparts, as was the transcriptional activity of Cg-p53.48
Significantly, we failed to discover a BH3-only homolog in C. gigas, nor has one been identified in the entire Mollusca phylum.33, 34 BH3-only proteins participate in the apoptotic response to various stressors.46 As such, the absence of a BH3-only homolog may imply a less-complex regulatory network in C. gigas, or in all Mollusca species. A simpler network might expedite the process of apoptosis, particularly in species that lack adaptive immunity49 and extrinsic apoptosis.50 Alternatively, it might also indicate a less stable apoptotic regulatory system. Either way, the impact of missing BH3-only proteins on apoptosis and the environmental adaptation mechanism of C. gigas and mollusks is of future interest.
Apoptosis is a crucial host defense mechanism.51 Our confirmation of mitochondrial apoptosis in C. gigas and the regulatory functions of oyster Bcl-2 family members, along with the stimulus-induced expression differences of the oyster Bcl-2 family genes under various stresses, support the extensive involvement of mitochondrial apoptosis in the environmental adaptation process of C. gigas. However, much effort will be needed to clarify the exact role of mitochondrial apoptosis in the response to various stressors.
In conclusion, the present study characterized the conservation and divergence of mitochondrial apoptosis in the Pacific oyster C. gigas. However, it is important to point out that many functional experiments were conducted in yeast or human cell lines as molecular tools in this study given the limitation of our experimental system. The limitation that is general to many non-model organisms is that cell lines and cell line-based research such as gene overexpression, protein–protein interaction is still challenging. However, despite these limitations, we found most events in C. gigas mitochondrial apoptosis displayed great similarity to that in vertebrate and S. mediterranea including MOMP and cytochrome c release. On the other hand, the absence of BH3-only proteins and the lack of a domain-intact APAF-1 homolog in Pacific oyster were indicative of pathway diversity in invertebrates. Continued investigation in other invertebrates will aid in our understanding of mitochondrial apoptosis pathway evolution.
Materials and methods
Chemicals, plasmids, small-interfering RNAs, and antibodies
H2O2 was purchased from Sangon (Shanghai, China). Cytochrome c from equine heart was purchased from Solarbio (Beijing, China), and C. gigas cytochrome c was synthesized by Chemgen Biotechnology (Shanghai, China). dATP was obtained from Tiangen (Beijing, China). The Z-LEHD-FMK and PFT-α inhibitors were purchased from BioVision (Milpitas, CA, USA) and Beyotime (Jiangsu, China), respectively. The pGADT7, pGBKT7, and pEGFP-N1 plasmids were purchased from Takara (Shiga, Japan). pCMV-N-Myc and pCMV-N-FLAG plasmids were obtained from Beyotime and the pYES2/CT from Invitrogen (Carlsbad, CA, USA). The pRL-TK and pGL3-basic plasmids were both from Promega (Madison, MI, USA). Small-interfering RNAs targeting Cg-Bak (Cg-Bak1 sense: 5'-GGACGUGAUCAGGAACUUUTT-3', anti-sense: 3'-AAAGUUCCUGAUCACGUCCTT-5'; CgBak2 sense: 5'-GGCGAUAUGCCGAUGAAUUTT-3', anti-sense: 3'-AAUUCAUCGGCAUAUCGCCTT-5'; CgBak3 sense: 5'-GGUCAUUGUCAGUCAUGUUTT-3', anti-sense: 3'-AACAUGACUGACAAUGACCTT-5'; scrambled negative control siRNA sense: 5'-UUCUCCGAACGUGUCACGUdTdT-3', anti-sense: 3'-ACGUGACACGUUCGGAGAAdTdT) and Cg-Bax (Cg-Bax1 sense: 5'-GCAGAGCUUUACGUUGCAUTT-3', anti-sense: 3'-AUGCAACGUAAAGCUCUGCTT-5'; Cg-Bax2 sense: 5'-CCUUUGGAAGGCACUCAAATT-3', anti-sense: 3'-UUUGAGUGCCUUCCAAAGGTT-5'; Cg-Bax3 sense: 5'-GCAGAGUGGGAUGUCUAUUTT-3', anti-sense: 3'-AAUAGACAUCCCACUCUGCTT-5') were obtained from GenePharma (Shanghai, China). Antibodies against FLAG and EGFP were purchased from Sigma (St. Louis, MO, USA). Myc antibody was from Roche (Basel, Switzerland). Antibody against cytochrome c was synthesized by Chemgen Biotechnology. Peroxidase-labeled mouse IgG secondary antibody was purchased from KPL (Gaithersburg, MD, USA).
Oyster and primary hemocyte culture
Pacific oysters averaging 7 cm in shell height were obtained from a local farmer in Qingdao, China, and acclimatized in tanks with 20±0.5 °C, pH 8±0.3 seawater. Primary hemocyte culture was performed as previously described with slight modifications.52 In brief, hemocytes were withdrawn from the pericardial cavity using a sterile 21-gauge needle attached to a 1 ml syringe containing 0.1–0.2 ml ice-cold filtered sterile seawater (FSW) supplemented with 2 g/l glucose. The cells were plated into 6-well plates, adjusted to ~2 × 106 per well, and allowed to adhere for 30 min at room temperature. Hemolymph then was removed and Leibovitz L-15 medium (Sigma) supplemented with additives52 (including 0.54 g/l KCl, 20.2 g/l NaCl, 0.6 g/l CaCl2, 3.9 g/l MgCl2, 1 g/l MgSO4, 20.8 g/l glucose, 220 μg/ml streptomycin, 100 μg/ml gentamicin, 100 μg/ml penicillin, and 0.1 μg/ml amphotericin B) was added to suspend the cells before culturing at 18 °C.
Viral challenge, vibrio challenge, heat shock, air exposure, and UV irradiation
Viruses were obtained as previously described.53 Live V. alginolyticus were suspended with sterilized PBS and adjusted to 5 × 107 cells/ml. Before challenge, a small hole was made, using a sand-saw, on the edge of the oysters’ shells to accommodate the injection. Three days later, 0.1 ml viral homogenate, the V, alginolyticus suspension or PBS was injected into the oysters. Six individuals from each challenge group were randomly sampled at 0, 3, 6, 12, 24, 48, and 72 h after injection and the hemocytes were collected. For heat shock treatment, oysters were placed in tanks with 35 °C seawater for 1 h, transferred back to 25±0.5 °C seawater, and then, six individuals from each group (treated and untreated) were sampled 0, 1, 3, 6, 12, and 24 h later. For air exposure experiment, oysters were placed in a tank without seawater at 20±1 °C and then tissues were collected from six individuals in each group (treated and untreated) at 1, 3, 5, 7, 9, 10, and 11 days after exposure. For UV irradiation, cell culture medium was reduced to 500 μl prior to irradiation. Hemocytes were then exposed to UV light (15 W, Philips, Netherlands) for 20 min, the media volume restored to 1 ml, and cells were sampled at distinct time points based on the analysis. Hemocytes from six independent wells were sampled as experimental replicates at each time point.
Transmission electron microscopy
TEM analysis of oyster hemocytes was performed following a previous study.29 Hemocyte suspensions (1 × 106 cells) were centrifuged at 500 × g for 8 min at 4 °C, and the supernatant was discarded. Samples were fixed in 3% glutaraldehyde solution for 1 day at 4 °C. After 3 washes with 0.4 M cacodylate buffer, the cells were post-fixed with a solution of 1% osmium tetroxide for 1 h at 4 °C. Then, the cells were washed twice in 0.4 M cacodylate buffer. After dehydration in successive baths of ethanol and two baths of propylene oxide, samples were progressively impregnated and embedded in Epon. After polymerization at 60 °C, semi-thin sections were cut to 1 mm thickness for quality control and then to 80–85 nm for examination on a Leica Ultracut (EM UC6), floated onto copper EM grids, and stained with uracil acetate/Fahmys lead citrate. The sections were examined using a transmission electron microscope (H-7000, Hitachi, Japan).
Real-time PCR analysis
Total RNA from tissues and cells were extracted using TRIzol (Invitrogen) following the manufacturer’s instructions. RNA integrity was assessed using agarose gel electrophoresis, and purity was estimating according to the A260/280 absorption ratio measured using a NanoDrop 2000 Spectrophotometer (Thermo Fisher Scientific, Sunnyvale, CA, USA). cDNA was synthesized by reverse transcription with the PrimeScript RT reagent kit with gDNA Eraser (TaKaRa, Shiga, Japan). Real-time PCR was carried out on an ABI 7500 Fast Real-Time PCR System (Applied Biosystems, Foster City, CA, USA) using 2 × SYBR Ex Taq mix (TaKaRa) according to the manufacturer’s protocol. Cg-GAPDH was used as an internal control for expression analysis in response to OsHV-1, heat shock and air exposure.23, 45 Cg-β-actin was used as an internal control in UV light irradiation analyses.25
Mammal cell cultures and transfection
HEK293T cells (ATCC, Manassas, VA, USA) were cultured in high-glucose Dulbecco’s Modified Eagle’s Medium (HyClone, Logan, UT, USA). HeLa cells were cultured in modified Roswell Park Memorial Institute (RPMI)-1640 medium (HyClone). Both media were supplemented with 10% fetal bovine serum (HyClone), penicillin (100 U/ml), and streptomycin (100 U/ml). Cells were maintained at 37 °C in a humidified atmosphere of 5% CO2. Plasmid transient transfection was performed with Lipofectamine 3000 (Invitrogen) according to the manufacturer’s protocol.
Yeast death assays
pYES2/CT constructs carrying distinct fragments with or without pADH with the indicated inserts were transformed into S. cerevisiae, which was then cultured on the appropriate non-inducing medium as previously described.18 Isolated colonies were suspended in water, diluted 10-fold, and then plated on inducing and non-inducing medium. Plates were imaged ~3 days later.
Yeast two-hybrid and co-IP assays
The yeast two-hybrid system was carried out using Clontech Matchmaker Gold Yeast Two-Hybrid System (TaKaRa). pGADT7 and pGBKT7 carrying various oyster gene fragments were transformed into the Y187 and Gold yeast strains, respectively. Y187 cells and Gold cells were cultured onto selective plates with synthetically defined medium (SD) lacking leucine (SD/-Leu) or tryptophan (SD/-Trp) separately. Three days later, positive yeast strains on SD/-Leu and SD/-Trp were collected and hybridized in 2 × yeast extract peptone dextrose (YPDA) medium and selected on double drop-out SD/-Leu/-Trp medium. The blue hybridized clones growing on quadruple drop-out SD/-Ade/-His/-Leu/-Trp medium supplemented with X-α-Gal and Aureobasidin A (TaKaRa) indicated potential protein interactions. For co-IP assays, HEK293T cells transfected with plasmids expressing the FLAG and Myc tags were harvested at 30 h post-transfection with cell lysis buffer (Beyotime). Input samples were prepared from the cell lysate. The remaining lysate was mixed with anti-FLAG M2 magnetic beads (Sigma-Aldrich) and shaken gently on a roller shaker for 1–2 h. Subsequently, the magnetic beads were washed three times with cell lysis buffer and incubated with 2 × SDS-PAGE loading buffer (TaKaRa) for 8 min at 100 °C to elute the bound protein. Then, the beads were removed and immunoprecipitated proteins were analyzed using western blotting.
Extraction of mitochondrial and cytoplasmic proteins and western blot analysis
Mammalian and oyster mitochondria were isolated using a Cell Mitochondria Isolation Kit (Beyotime) following the manufacturer’s protocol. The mitochondrial or cytoplasmic proteins were extracted from the prepared fractions with lysis buffer. For western blotting, proteins were resolved by 12% SDS-PAGE and transferred onto a 0.45 nm pore nitrocellulose membrane with the use of Semi-dry blotter (GenScript, Jiangsu, China). The membrane was then blocked with TBST (20 mmol/l Tris-HCL, 150 mmol/l NaCl, and 0.05% Tween-20) containing 5% skimmed milk at room temperature for 1 h, and then incubated with the appropriate antibodies at 4 °C overnight, washed three times with TBST, incubated with peroxidase-labeled secondary antibodies at room temperature for 1 h, and finally washed five times with TBST. Western Lightning Plus-ECL substrate (PerkinElmer, Waltham, MA, USA) was then added to membranes, which were exposed to X-OMAT AR X-ray film (Eastman Kodak, Rochester, NY, USA).
pEGFP-N1 carrying distinct gene fragments were transfected into HeLa cells. HeLa cells were rinsed once with PBS 24 h later and then stained with 2 mg/ml Hoechst 33342 (Invitrogen) for 10 min at 37 °C. Subsequently, the cells were washed twice with PBS, stained with Alexa Fluor 594 (Life Technologies, Carlsbad, CA, USA) for 15 min at 37 °C, washed three times with PBS, and then cultured in modified RPMI-1640 medium without fetal bovine serum. The visualization of protein subcellular localization was performed by confocal microscopy (Carl Zeiss, Oberkochen, Germany).
Inhibitor treatments on oyster hemocytes
Cell culture medium was replaced with fresh medium containing one of the inhibitors: PFT-α (100 μM), Z-LEHD-FMK (35 μM), or siRNA (30 μg/ml). Cells were incubated with PFT-α or Z-LEHD-FMK for 1 h, or siRNA for 24 h before UV light irradiation.
Transcription activity assay
HEK293T cells were used to examine Cg-p53 transcriptional activity. The region ~2 kb upstream of the Cg-Bak, Cg-Bax, Cg-Bcl-2, and Cg-Bcl-xl start codons were considered as potential promoter regions and cloned to the pGL3-basic luciferase reporter plasmid to generate the Cg-Bak-Luc, Cg-Bax-Luc, Cg-Bcl-2-Luc, and Cg-Bcl-xl-Luc plasmids. Cells were co-transfected with varying amounts of pRL-TK, luciferase reporter, pCMV-N-Myc-Cg-p53, and pCMV-N-Myc plasmids and luciferase activity was measured using Dual-Luciferase Reporter Assay System (Promega) 24 h after transfection.
Assessment of caspase activity and apoptosis
For caspase 3 and caspase 9 activity assays, HEK293T cells or oyster hemocytes were collected, lysed, and the concentration of total protein measured by Bradford method. Caspase activity was then monitored with the Caspase 3 Activity Assay Kit (Beyotime) and Caspase 9 Activity Assay Kit (Beyotime). Annexin V/PI immunostaining was used to assess apoptosis in cells using the FITC-Annexin V Apoptosis Detection Kit (BD Biosciences, San Jose, CA, USA) according to the manufacturer’s instructions. In brief, cells were washed with PBS, suspended with binding buffer, stained with FITC-Annexin V and PI, and analyzed with a FACS Calibur flow cytometer (BD).
JC-1 assay for MMP
The MMP of oyster hemocytes was evaluated with the JC-1 Mitochondrial Membrane Potential Detection Kit (Beyotime) according to the manufacturer’s protocol. Briefly, hemocytes that mixed with 10 μM CCCP for 20 min before JC-1 staining served as a positive control. Hemocytes in each well were collected and resuspended with 1 ml modified L-15 medium and then mixed with JC-1 staining solution. Twenty minutes later, the cells were rinsed twice with 1 × staining buffer and analyzed with a Varioskan Flash multimode reader (Thermo Fisher Scientific).
Data were analyzed by Student’s t-test or one-way ANOVA to determine the differences among different groups. P<0.05 was considered statistically significant.
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This study was supported by the National Basic Research Program of China (973 Program, No. 2010CB126402), the National Natural Science Foundation of China (31302219), the National High Technology Research and Development Program (863 program, 2012AA10A405), the Earmarked Fund for Modern Agro-industry Technology Research System (CARS-48), and Taishan Scholars Climbing Program of Shandong. This research was supported by the National Natural Science Foundation of China (31530079), the Strategic Priority Research Program of 'Western Pacific Ocean System: Structure, Dynamics and Consequences' (Grant No. XDA11000000), Technological Innovation Project Financially Supported by Qingdao National Laboratory for Marine Science and Technology (2015ASKJ02-03) and the Earmarked Fund for Modern Agro-industry Technology Research System (CARS-48).
The authors declare no conflict of interest.
Edited by G Melino
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Li, Y., Zhang, L., Qu, T. et al. Conservation and divergence of mitochondrial apoptosis pathway in the Pacific oyster, Crassostrea gigas. Cell Death Dis 8, e2915 (2017). https://doi.org/10.1038/cddis.2017.307
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