Programmed cell death, which occurs through a conserved core molecular pathway, is important for fundamental developmental and homeostatic processes. The human iron–sulfur binding protein NAF-1/CISD2 binds to Bcl-2 and its disruption in cells leads to an increase in apoptosis. Other members of the CDGSH iron sulfur domain (CISD) family include mitoNEET/CISD1 and Miner2/CISD3. In humans, mutations in CISD2 result in Wolfram syndrome 2, a disease in which the patients display juvenile diabetes, neuropsychiatric disorders and defective platelet aggregation. The C. elegans genome contains three previously uncharacterized cisd genes that code for CISD-1, which has homology to mitoNEET/CISD1 and NAF-1/CISD2, and CISD-3.1 and CISD-3.2, both of which have homology to Miner2/CISD3. Disrupting the function of the cisd genes resulted in various germline abnormalities including distal tip cell migration defects and a significant increase in the number of cell corpses within the adult germline. This increased germ cell death is blocked by a gain-of-function mutation of the Bcl-2 homolog CED-9 and requires functional caspase CED-3 and the APAF-1 homolog CED-4. Furthermore, the increased germ cell death is facilitated by the pro-apoptotic, CED-9-binding protein CED-13, but not the related EGL-1 protein. This work is significant because it places the CISD family members as regulators of physiological germline programmed cell death acting through CED-13 and the core apoptotic machinery.
The core programmed cell death pathway is highly regulated to maintain normal developmental and homeostatic processes. This well-studied pathway, composed of pro-survival Bcl-2, pro-death APAF-1 and pro-death caspases, is regulated in a cell- and stimulus-dependent manner. One of the core principles regulating this pathway involves mutually exclusive interactions of Bcl-2 with the BH3 domain (Bcl-2 homology region 3) pro- or anti-apoptotic proteins that modulate Bcl-2 activity. The iron–sulfur (2Fe-2S) protein NAF-1/CDGSH iron sulfur domain 2 (CISD2; nutrient autophagy factor) was identified as a protein that binds to Bcl-2 at the ER . Additionally, the displacement of NAF-1 from Bcl-2 binding occurs via the Endoplasmic Reticulum (ER) localized BH3-only protein Bik . These results led to the hypothesis that the Bcl-2:NAF-1 complex at the ER plays a key role in regulating apoptosis and autophagy in mammalian cells [2,3,4]. Mapping of the binding interface between Bcl-2 and NAF-1 subsequently revealed that NAF-1 binds to Bcl-2 at the same site that a BH3-only protein would . Further support for the involvement of NAF-1 in autophagy/apoptosis regulation comes from studies in cancer cell lines, xenograft tumors and the null NAF-1 mouse model, in which NAF-1 dysfunction led to the activation of apoptosis . However, the role NAF-1 has in programmed cell death and whether this protein regulates apoptosis via binding to Bcl-2 is not understood [1, 3, 4].
The CISD protein family includes NAF-1/CISD2, the mitochondrial outer membrane protein mitoNEET/CISD1 and the mitochondrial protein CISD3/Miner2 [6,7,8,9]. Phenotype analyses indicate that the NAF-1/CISD2 and mitoNEET/CISD1 proteins are multifunctional and have various cellular roles including those involved in mitochondria function and cell proliferation [6, 10,11,12]. In humans, a mutation in CISD2 results in Wolfram syndrome 2 disease, an autosomal recessive disorder characterized by early onset of juvenile diabetes mellitus, optic atrophy, deafness, renal abnormalities and neuropsychiatric disorders [13,14,15,16,17,18,19]. Relative to mitoNEET and NAF-1, much less is understood about the function of Miner2/CISD3 because in-depth phenotype analysis associated with CISD3 gene dysfunction has not been conducted.
Many biological processes, including apoptosis, have been elucidated from the genetic and cell biological analyses in the Caenorhabditis elegans (C. elegans) model system [20, 21]. Here we use the C. elegans genetic system to study the function of the cisd gene family. The C. elegans genome contains three previously uncharacterized cisd genes (cisd-1, cisd-3.1 and cisd-3.2). The cisd-1 gene codes for a protein that shows homology to the vertebrate mitoNEET/CISD1 and NAF-1/CISD2, and the cisd-3.1 and cisd-3.2 genes code for proteins that show homology to vertebrate CISD3 . Using CRISPR technology, we developed a cisd-1p::GFP reporter and determined that the cisd-1 promoter drives expression in the hermaphrodite germline. The C. elegans hermaphrodite gonad is a U-shaped structure that consists of somatic cells and the germline, which produces sperm and oocytes . During the process of oogenesis, some cells will naturally undergo apoptosis; this process is referred to as germline physiological apoptosis . The analysis of germline physiological apoptosis within C. elegans provides a model for cell death mechanisms needed to maintain the structure and function of an organ. In addition to physiological cell death, apoptosis within the germline will increase in response to various stresses (e.g., DNA damage) or defects in synapsis during meiosis [20, 23]. The mechanisms involved in physiological cell death and environmentally induced cell death within the C. elegans germline involve the core apoptotic machinery (CED-9, CED-4 and CED-3) . Although many pioneering studies have been done using C. elegans to reveal the genetic mechanisms regulating apoptosis, questions still remain regarding the regulation of physiological germline apoptosis [20, 25, 26].
Here, we determined that disruption of cisd-1 gene function, using RNA interference (RNAi), or mutant alleles [cisd-1(tm4993) deletion mutant, cisd-1(pnIs27) insertion mutant] led to germline abnormalities including an increase in the number of cell corpses and distal tip cell migration defects. RNAi knock-down of cisd-3.1 or cisd-3.2 resulted in similar phenotypes indicating functional overlap within the cisd gene family. Disruption of ced-3/caspase or ced-4/APAF-1 function, or the gain-of-function ced-9(n1950) mutation reduced the number of cell corpses in the germline of the cisd-1(tm4993) animal. Additionally, disruption of ced-13, which codes for a pro-apoptotic, BH3 (Bcl-2 homology region 3) protein that physically interacts with the anti-apoptotic CED-9/Bcl-2 protein, significantly reduced the number of germ cell corpses observed in the cisd-1(tm4993), cisd-3.1(RNAi) and cisd-3.2(RNAi) animals. These results show that the C. elegans cisd genes function in the process of apoptosis and place the CISD protein family as regulators of physiological germline programmed cell death with CED-13.
Disruption of the cisd genes impact germline structure and germ cell survival
The C. elegans genome contains three previously uncharacterized cisd genes (cisd-1, cisd-3.1 and cisd-3.2) that code for the CISD proteins (Figure S1a). The cisd-1 gene codes for two isoforms (Figure S1b) that show homology to the vertebrate mitoNEET/CISD1 and NAF-1/CISD2 (Figure S1c), and the cisd-3.1 and cisd-3.2 genes code for proteins that show homology to vertebrate CISD3 (Figure S1d) . All three of the CISD proteins contain putative 2Fe-2S domain(s) with their signature CDGSH motif (Figure S1a). To study the cisd-1 gene function in the context of a whole organism, we used the C. elegans genetic mutant cisd-1(tm4993). The cisd-1(tm4993) mutant contains a 316 basepair (bp) deletion that removes a significant portion of the coding region of both cisd-1a and cisd-1b. The cisd-1 mRNA is not detected, by quantitative reverse transcriptase-PCR (qRT-PCR), in the cisd-1(tm4993) animal indicating that the tm4993 allele is a null mutation (Figure S2a). The cisd-1(tm4993) animals displayed various germline defects (Fig. 1). First, the number of differentiated oocytes is reduced in the cisd-1(tm4993) mutant relative to N2 wild-type animals (Figs. 1a, d). Additionally, the majority of cisd-1(tm4993) animals display a germline distal tip cell migration defect (referred to as a Mig phenotype) . The Mig phenotype is observable in L4 larvae (Fig. 1b) and young 1-day old adults (Figs. 1c, e). The reduced number of oocytes and increased Mig phenotype was also observed within the germline of cisd-1(RNAi) animals (Figure S3a, b). Note that RNAi effectively reduced cisd-1 gene function as determined by qRT-PCR (Figure S2b). The germline defects associated with the cisd-1(tm4993) allele do not lead to complete sterility but there is a reduction in the number of eggs laid relative to N2 control (Fig. 1f). The total number of offspring for the cisd-1(tm4993) hermaphrodite relative to the N2 control is significantly lower (cisd-1(tm4993) = 193.8 ± 17.7, N2 = 341.8 ± 15.8, P < 0.001, two-tailed unpaired t-test). Combined, these data support the idea that cisd-1 function is important for normal germline function.
Relative to mitoNEET and NAF-1 in mammalian systems, much less is understood about the function of Miner2/CISD3. Here, we used RNAi to knock-down cisd-3.1 and/or cisd-3.2 gene function, in both the N2 wild-type and cisd-1(tm4993) animals to determine if such impacts the germline structure and if the phenotype is more severe when more than one cisd gene is dysfunctional. Knock-down of the cisd-3.1 and/or cisd-3.2 gene function reduced the number of differentiated oocytes within the germline of 1-day old adults, relative to N2 wild-type control animals (Figs. 2a (left panel), b). The combination of cisd-3.1 and/or cisd-3.2 knock-down with the cisd-1(tm4993) mutation further reduced the number of mature oocytes relative to the cisd-1(tm4993) single mutant (Fig. 2b, gray dot plot). The disruption of cisd-3.1 or cisd-3.2 gene function also resulted in a Mig phenotype (Figs. 2a (right panel), c). Relative to the cisd-1(tm4993), the combination of cisd-3.1 and/or cisd-3.2 knock-down with the cisd-1(tm4993) mutation did not further increase the number of animals displaying the Mig phenotype relative to the cisd-1(tm4993) (Fig. 3c, gray bars); this is likely due to the fact that the penetrance of the Mig phenotype is already high when a cisd gene is disrupted. These results indicate that the cisd gene family has a role in germline structure and function and the cisd genes have overlapping functions. Note that RNAi effectively reduced cisd-3.1 and cisd-3.2 gene function as determined by qRT-PCR (Figure S2b).
Our results indicate that cisd dysfunction leads to germline defects. Thus, we wanted to examine if cisd-1 is expressed within the germline. Transgenic genes are known to be silenced within the germline . However, recently developed CRISPR methods have been shown to be effective in producing GFP transcriptional reporters for genes known to be expressed within the germline . We used this approach to produce the cisd-1(pnls27 [GFP^SEC^3xFlag::cisd-1]) transcriptional reporter strain (PM154) (Fig. 3a). This methodological approach also produces an insertion mutant, which can be used to verify phenotypes associated with cisd-1 dysfunction (Fig. 3a) . The cisd-1 mRNA, as detected by qRT-PCR analysis, is significantly reduced in the cisd-1(pnIs27) mutant suggesting this allele is a null mutation (Figure S2a). The cisd-1(pnIs27) animals showed GFP expression in the germline of L4 (Fig. 3b) and young adults (Fig. 3c). The GFP expression was also observed in embryonic blastomeres, and the muscle and intestinal cells within larvae and young adults (data not shown). Similar to the cisd-1(tm4993) mutant, the cisd-1(pnIs27) animals had a reduced number of mature oocytes (Figure S3c) and a reduction in progeny relative to control N2 wild-type animals (Figure S3d). These data provide further support that CISD-1 functions within the C. elegans germline.
Reduction of cisd gene family function increases cell corpses in the germline
Previously we showed that breast cancer cell lines with suppressed NAF-1/CISD2 expression (grown in culture or xenograft tumors) display features of activated apoptosis . Furthermore, through the use of synthetic peptides the NAF-1/CISD2 protein was shown to interact with Bcl-2 . However, it is unclear what role NAF-1/CISD2 has in the apoptotic pathway. Given that the knock-down of cisd function in C. elegans causes germline defects, including the Mig phenotype, which is associated with mutations in genes that have a role in cell corpse engulfment following germline apoptosis (e.g., ced-5, ced-10) [31,32,33], we asked if the cisd genes function during the physiological germline programmed cell death process in C. elegans. Using differential interference contrast (DIC) microscopy to directly visualize cell corpses, we determined that the cisd-1(tm4993) (Figs. 4a, b) and cisd-1(pnls27) (Figure S3e) animals have an increased number of cell corpses in the germline relative to control wild-type animals. To confirm and further examine this finding, we used established programmed cell death reporters that mark distinct time points in the process of programmed cell death . The ACT-5::YFP marker is expressed in somatic sheath cells and marks pre-disc corpses; this is used as a reporter for the early stages of apoptosis . The CED-1::GFP marker is expressed in cells that have initiated the process of engulfment . The vital dye acridine orange stains internalized apoptotic cells [24, 37]. Using these three different approaches, we confirmed that the cisd-1(tm4993) animal has a significantly higher number of cell corpses in the germline relative to respective controls (Figs. 4c–f). Animals defective in cell corpse engulfment (e.g., dyn-1(ky51), ced-1(e1735), and vps-34(RNAi)) have gonads that accumulate cell death corpses when visualized by DIC microscopy but are defective for acridine orange staining indicating that these genes have a functional role in cell corpse processing [20, 37]. Within the gonad of the cisd-1(tm4993) animal, the cell corpses, as visualized by DIC microscopy, were positive for acridine orange suggesting that CISD-1 is not involved with cell corpse processing (Figs. 4c, f). To confirm that the cisd-1 mutant does not display cell corpse processing defects, we assayed for the persistence of cell corpses in newly hatched cisd-1(tm4993) L1 larvae and embryos at the bean or comma stage of development, relative to N2 wild-type and the ced-1(e1735) positive control animal. The N2 wild-type and cisd-1(tm4993) L1 larvae did not contain cell corpses that persisted into the L1 larvae stage (30 animals assayed), whereas the positive control ced-1(e1735) animal did show the persistent cell corpse phenotype. Additionally, there was not a significant difference between the number of cell corpses observed within the N2 wild-type and cisd-1(tm4993) comma-staged embryo (12.1 ± 1.3, 12.1 ± 1.0, P > 0.05); the positive control ced-1(e1735) embryo did have a significantly higher number of cell corpses as expected (20.0 ± 2.4, P < 0.001). Together, these data indicate that the cisd-1(tm4993) mutant has a defect in the regulation of physiological apoptosis and that this defect is not associated with a defect in the cell corpse engulfment process.
We used the ACT-5::YFP and CED-1::GFP reporters to examine if knock-down of cisd-3.1 and/or cisd-3.2 function impacts physiological programmed cell death within the germline. The cisd-3.1(RNAi), cisd-3.2(RNAi), and cisd-3.1(RNAi); cisd-3.2(RNAi) animals had an increased number of cell corpses within the germline relative to control (Figs. 5a (left panel), b; Figure S4a left panel, b). The combination of cisd-3.1 and/or cisd-3.2 knock-down with the cisd-1(tm4993) mutation did not further increase in the number of cell corpses relative to cisd-1(tm4993) (Figs. 5a (right panel), c; Figure S4a right panel, c). Our data support the idea that the cisd gene family functions in the process of physiological germline apoptosis.
The increased germline cell death in the cisd-1 mutant is mediated through the core apoptotic machinery and depends on CED-13 function
The core apoptotic machinery in C. elegans is coded by the ced-3, ced-4 and ced-9 genes that are required for the regulation of programmed cell death during embryogenesis and within the germline [20, 26]. The ced-3 gene encodes a caspase, the ced-4 gene is orthologous to the APAF-1 gene encoding the apoptotic protease-activating factor 1 (Apaf-1) and the ced-9 gene is orthologous to the BCL-2 gene encoding the apoptotic regulator (Bcl-2). The CED-9 protein functions to prevent cells from dying by binding and regulating CED-4; this will ultimately impact the ability for CED-3 to cleave cellular proteins. We examined if the increased germline apoptosis observed in the cisd-1(tm4993) mutant and cisd-1(RNAi) animal is through the core apoptotic machinery. Using the ACT-5::YFP or CED-1::GFP programmed cell death reporters, we determined that ced-3 function is required for the increase in programmed cell death observed in animals with cisd-1 dysfunction (Fig. 6, Figure S5, Figure S6). The cisd-1(tm4993); ced-3(RNAi) animal had a significantly reduced number of cell corpses relative to that observed in the cisd-1(tm4993) (Figs. 6a, b). Similar results were observed in the cisd-1(RNAi); ced-3(RNAi) animal using the ACT-5::YFP (Figure S5a, b) or in the cisd-1(tm4993); ced-3(RNAi) using the CED-1::GFP reporter strain (Figure S6a, b). Furthermore, there was a significant decrease in the number of cell corpses in the cisd-1(RNAi); ced-4(n1162) animal relative to the cisd-1(tm4993) mutant (Figure S6a, c). Combined, these results indicate that the increase in cell corpses observed in the cisd-1(tm4993) mutant or cisd-1(RNAi) animal required the activity of CED-3 and CED-4.
During our analysis, we noticed that the knock-down of ced-3 function by RNAi did not suppress the Mig phenotype within the germline of the cisd-1(tm4993) animal (Figure S7). Others have shown that ced-5 or ced-10 dysfunction results in a Mig phenotype . The knock-down of ced-5 or ced-10 via RNAi in the cisd-1(tm4993) mutant did not further increase the Mig phenotype relative to the single mutant (Figure S7). Together, these results suggest that the increased cell corpses within the germline and the germline Mig phenotype are a result of distinct dysfunctions in the cisd-1(tm4993) animal.
The CED-9 protein functions to prevent cells from dying. Thus, the ced-9(n1950gf) gain-of-function mutant has been instrumental in examining the prevention of cell deaths within the embryo  or germline [20, 24]. Using the ACT-5::YFP reporter, we tested if the ced-9(n1950gf) allele would reduce the number germline cell death in the cisd-1(tm4993) animals. The cisd-1(tm4993); ced-9(n1950gf) animal had a significantly reduced number of cell corpses relative to cisd-1(tm4993) animals (Figs. 6a, c). The number of cell corpses was not completely eliminated in the ced-9(n1950gf); cisd-1(tm4993) mutant, which is in line with the previous reports that physiological germline apoptosis is not completely prevented by the ced-9(n1950gf) mutation [20, 24]. These data provide further evidence that the increased cell death observed in the cisd-1(tm4993) animals is due to altered regulation of the core apoptotic machinery.
In C. elegans, the egl-1 and ced-13 genes code for two pro-apoptotic, BH3 (Bcl-2 homology region 3) proteins that physically interact with and regulate the anti-apoptotic CED-9 protein [39,40,41]. Using the ACT-5::YFP reporter strain, we tested if ced-13(RNAi) or egl-1(RNAi) reduced the number of apoptotic cells within the germline of cisd-1(tm4993) animals. The number of cell death corpses within the germline was not significantly different in the cisd-1(tm4993); egl-1(RNAi) animal relative to the cisd-1(tm4993) animal (Figure S8). This is consistent with the idea that loss-of-function egl-1 does not impact physiological germline cell death . However, the cisd-1(tm4993); ced-13(RNAi) animal had a significant reduction in cell death corpses relative to the cisd-1(tm4993) animal (Fig. 7). Furthermore, ced-13(RNAi) significantly reduced the number of cell death corpses within the germline of cisd-3.1(RNAi) and cisd-3.2(RNAi) animals (Fig. 7). To confirm that ced-13 dysfunction suppressed the increased programmed cell death observed within the cisd-1(tm4993) germline, we crossed in the ced-13(sv32) loss-of-function allele into the cisd-1(tm4993) mutant. The cisd-1(tm4993); ced-13(sv32) double mutant had a significant reduction in cell death corpses within the germline relative to cisd-1(tm4993) animal (Figure S9). Combined, these data demonstrate that the cisd gene family could function as regulators of physiological germline programmed cell death acting through ced-13 function.
Disruption of the cisd gene family in C. elegans resulted in various germline defects including increased physiological apoptosis and DTC migration defects. A previous study examining the phenotypes associated with disrupted cisd gene function in mammalian cells also noted an increase in apoptosis as determined by biochemical assays, histochemistry and annexin staining, but did not determine whether this activation directly involved core programmed cell death members such as BCL-2 . Here we demonstrate that the CISD family members play a pro-survival role in the process of apoptosis and that they function through the Bcl-2 family CED-9 and BH3 domain CED-13 but not through EGL-1. Furthermore, we show that the CISD-3 proteins in C. elegans have overlapping functions with CISD-1.
Given that the knock-down of any one of the cisd gene family members increased germline apoptosis, we propose that they have overlapping functions in C. elegans. Furthermore, we suggest that the CISD proteins work in a cooperative manner and that disruption of one member of the gene family alters that cooperativity. This idea is in line with the findings that NAF-1/CISD2 and mitoNEET/CISD1 physically interact and cooperate in their function in mammalian cells . Given that ced-3(RNAi), ced-4(n1162) and ced-9(n1950gf) suppressed the increased germline programmed cell death observed in cisd-1(tm4993) and/or cisd-1(RNAi) animals, we propose that CISD proteins function upstream of the core apoptotic machinery.
Figure 8 communicates our working model of how the CISD family functions within the physiological germline apoptosis pathway. This proposed model is based on our results presented here, the findings in the mammalian system that the NAF-1/CISD2 protein interacts with Bcl-2 at the same domain that the CED-13-related protein Bik binds , and that C. elegans CED-13 and CED-9 physically interact . This model is further supported by research showing that peptides specific for the BH3 domains of CED-13 or EGL-1 interact with CED-9 and that this interaction disassociates CED-9 from CED-4; presumably this would initiate apoptosis in vivo . We propose that the CISD proteins act in a pro-survival/anti-apoptotic manner, whereas CED-13 acts in a pro-apoptotic manner. CISD and CED-9 interaction could promote germ cell survival by inhibiting CED-9/CED-13 interaction (Fig. 8a). When the CISD function is disrupted, or in response to a signal initiating physiological cell death in the germline, there is an increase in CED-9/CED-13 interaction, which will in turn release CED-4 to activate CED-3 function (Fig. 8b). This model is in line with our finding that ced-13(RNAi) reduces the increased programmed cell death observed in the animals with disrupted cisd function. This is also consistent with previous studies in mammalian cell culture that show that NAF-1 binds to Bcl-2 at the same site in which BH3 domain proteins bind [1, 44].
We showed that cisd dysfunction resulted in various germline abnormalities, including DTC migration defects. The cisd-1(tm4993); ced-3(RNAi) animals continued to display the Mig phenotype in the absence of germline apoptosis. Thus, the DTC migration defect and increased germline apoptosis are likely due to alterations of two independent processes. Furthermore, it is likely that the cisd gene family in C. elegans is involved with various cellular processes. Other genes that cause a Mig phenotype when dysfunctional are involved with cell adhesion, pathfinding and cell death engulfment genes [31, 45]. It will be of interest to examine these non-apoptotic CISD functions in the context of pathways regulating cell migration.
As the pioneering work conducted in C. elegans to identify the molecular mechanisms regulating apoptosis within the embryo, subsequent studies have provided insights into germline programmed cell death [24, 26, 39, 46]. Although much work has been conducted, there remain questions regarding the regulation of physiological germline apoptosis. For example, it is not completely clear what triggers physiological apoptosis or why some germ cell fates undergo apoptosis and others do not. It will be of interest to examine these questions in the context of CISD function.
Materials and methods
Strains and culture conditions
Worms were raised and maintained at 20 °C on NGM (nematode growth media) and seeded with Escherichia coli(E. coli) (OP50) bacteria for food source, unless otherwise noted . The following strains were acquired from the Caenorhabditis Genetics Center (CGC): N2, CU1546 [ced-1p::ced-1::GFP + rol-6(su1006)], WS2170 [lim-1p::YFP::act-5 + unc-119(ed3)], KX89 [ced-4(n1162); lim-7p::ced-1::GFP + lin-15] , MT4770 [ced-9(n1950gf)], MT3608 [unc-13(ed42); ced-1(e1735)] and MD792 [ced-13(sv32)]. The ced-9(n1920) gain-of-function mutation is a point mutation affecting the ced-9 open reading frame resulting in a glycine to glutamate substitution . The ced-4(n1162) allele contains a premature stop codon . The MD792 strain [ced-13(sv32)] contains a deletion that removes the entire ced-13 coding region and 747-bp upstream of the ATG codon and 209-bp downstream of the TAA stop codon . The cisd-1(tm4993) mutant was obtained from the National BioResource Project (NBRP)  and back-crossed three times to N2 wild-type animals to produce strain PM147. The cisd-1(tm4993) mutant contains a 316-bp deletion that removes part of the coding region of both cisd-1a and cisd-1b (Figure S1b). The deletion removes a portion of intron 1 through exon 3 for cisd-1b and a portion of the 5′-UTR to exon 2 for cisd-1a. The deletion does not remove any coding region of adjacent genes. The PM147 strain was used to produce the following strains via genetically crossing with strains described above: PM151 [cisd-1(tm4993); ced-1p::ced-1::GFP + rol-6(su1006)], PM149 [cisd-1(tm4993); lim-1p::YFP::actin + unc-119(ed3)], PM153 [cisd-1(tm4993); ced-9(n1950gf); lim-1p::YFP::actin + unc-119(ed3)] and PM162 [lim-1p::YFP::actin + unc-119(ed3); ced-13(sv32); cisd-1(tm4993)]. The MT4770 [ced-9(n1950gf)] strain was used to produce strain PM152 [ced-9(n1950gf); lim-1p::YFP::actin + unc-119(ed3)]. The MD792 strain (ced-13(sv32)) was used to produce the PM161 strain [lim-1p::YFP::actin + unc-119(ed3); ced-13(sv32)]. The PM154 strain [cisd-1(pnls27[GFP^SEC^3xFlag::cisd-1])] was generated using the CRISPR technique as outlined below. The genotypes of strains produced by genetic crosses were verified by PCR (Table S1). DNA sequencing was also used to verify the genotypes of strains produced by crossing in the ced-9(n1950gf) allele.
CISD protein family sequence alignment
To examine sequence homology of the CISD proteins, multiple sequence alignments of the CISD protein sequences (FASTA format, Homo sapiens and C. elegans), were conducted using the Clustal Omega (1.2.4) web interface program . The output format parameters were set for Clustal alignment without numbers. The CISD-1 isoforms were aligned with the mitoNEET/CISD1 and Naf-1/CISD2 human protein sequences. The C. elegans CISD-3.1 and CISD-3.2 protein amino-acid sequences were aligned with the human Miner2/CISD3 protein sequence.
Generation of the cisd-1(pnls27) insertion and GFP reporter strain
We used the CRISPR/Cas9-based approach developed by Dickenson et al. to produce a GFP transcriptional reporter and insertion strain . The cisd-1 gene is predicted to code for two isoforms; cisd-1a contains two exons and cisd-1b contains three exons (Fig. 3a, Figure S1b). To disrupt both isoforms and produce a transcriptional GFP reporter for cisd-1, the CRISPR construct was designed such that the GFP insertion interrupted the first exon of cisd-1a and the second exon of cisd-1b. The Zhang’s lab CRISPR design tool website (crispr.mit.edu) was used to determine Cas9 target sequence. The protocol was designed for GFP^SEC^3xFlag insertion at 536-bp downstream of the start site. The pDD162 vector (Addgene plasmid #47549) was used to produce the cisd-1 Cas9-sg RNA (pCas9-sgc; cisd-1). The FP-SEC vector pDD282 (Addgene plasmid #66823) was used to produce the repair template plasmid for homologous recombination at the cisd-1 locus (GFP^SEC^3XFlag::cisd-1). The NEB Q5 Site-Directed Mutagenesis Enzyme Kit was used to produce the plasmid constructs. The approach for producing plasmid and microinjection mixtures were from the Goldstein Lab Self Excising Cassette Protocol . Synchronized 1-day old adult hermaphrodites were obtained and the DNA solution was micro-injected into the proximal gonad using an inverted compound microscope . After injection, worms were recovered and placed onto individual OP50 seeded plates and nematode candidates containing the GFP^SEC^3xFlag insertion were selected for by animals exhibiting hygromycin resistance and a roller phenotype . Three candidates were isolated; the PM154 strain, [cisd-1(pnls27 [GFP^SEC^3xFlag::cisd-1]) II], produced the most progeny with the roller phenotype and thus was used for analysis. The generated lines were verified by genotyping using PCR and DNA sequencing; the primer sequences used for this experiment are included in Table S1.
RNAi was conducted as previously described [53, 54]. The HT115 and RNAi E. coli strains were obtained from the Medical Research Council Geneservice, Source BioSciences (Cambridge, UK) or produced by our lab as outlined below [45, 55]. We produced RNAi strains, using standard DNA cloning techniques, to target cisd-1 or cisd-3.2 as these strains are not present in the Ahringer library. To construct the cisd-1 RNAi bacterial strain, 367 bp of the cisd-1 gene, which contained exons 2 and 3 and intron 2, was cloned into the L4440 vector to produce the plasmid pL440cW02B12.15. To construct the cisd-3.2 RNAi bacterial strain, 1564 bp of the cisd-3.2 gene, which encodes exons 1, 2 and 3 and introns 2 and 3, was cloned into the L4440 vector to produce plasmid pL440cY67D2.3. These DNA sequences were cloned so that the T7 promoter could generate the double-stranded RNA in the presence of IPTG (isopropyl-β-D-1-thiogalactopyranoside). The DNA within the plasmids were verified by DNA sequencing. The plasmids were transformed into HT115(DE3) bacteria. To conduct the RNAi experiments, animals were raised on NGM plates (0.5 g/ml IPTG, 200μg/ml ampicillin, 12.5μg/ml tetracycline) seeded with either HT115 control food (L4440 plasmid with no insert) or the E. coli strain for RNAi of the specified gene. Briefly, embryos were grown to 1-day old adulthood and the F1 embryos were transferred to fresh NGM IPTG plates seeded with the appropriate bacteria. The F1 embryos were raised on the RNAi food and analyzed at the developmental stage indicated for each experiment. The RNAi food to target par-6 was used as an internal control to test reagents effectiveness, because par-6(RNAi) leads to obvious phenotypes within the P0 and F1 generation (sterility, embryo lethality).
One-day old adult hermaphrodites were collected for mRNA isolation and RT-PCR as previously described [56, 57]. Briefly, mRNA was isolated using TRIzol Reagent (Life Technology, 15596026), NucleoSpin RNA Clean-up (Machenerey-Nagel, 740948-50) and TURBO DNA-freeTM kit (Life Technology, AM1907) reagents. The complementary DNA was generated using the SuperScript III synthesis system (Invitrogen, 18080-051). The quantitative RT-PCR was carried out using a StepOnePlus real-time PCR system (Applied Biosystems) and Fast SYBR Green Master Mix (Applied Biosystems, 4385612). The mRNA level of Y45F10D.4 was used for normalization . The average of three technical replicates was used for each experiment and the three independent biological replicates were statistical analyzed using one-way analysis of variance (ANOVA).
Germline phenotype analysis
The number of progeny produced by cisd-1(tm4993) and cisd-1(pnIs27) mutants, relative to N2 control, was determined as previously described . At least four synchronized animals were collected at the L4-to-adult molt, placed as individuals onto a NGM plate and allowed to lay eggs over a 24-h period. The adult worms were moved every 24 h and the progeny produced during each 24-h interval were counted after hatching. Animals were examined until no progeny were produced. To examine the anatomy and morphology of the hermaphrodite gonad, DIC microscopy was used to visualize the gonad within L4 larvae and 1-day old adults; only gonads that were completely visible were scored [24, 34]. Briefly, the proximal gonad arm was examined for the number of maturing oocytes by counting the oocytes from the primary oocyte to the region in the germline where the germ cells are in a non-linear arrangement (near the turn). The animals were scored as having a distal tip cell migration (Mig) defect if the morphology of the gonad was abnormal due to extra turns or abnormal turning was observed. For each experiment, at least three independent experiments were completed.
Programmed cell death assays
To quantify the germ cell corpses, synchronized L4 larvae were collected and the germline was examined 48 h later. The cell corpses within the germline were counted using DIC microscopy or fluorescent microscopy to visualize reporter strains or acridine orange staining [24, 34]. Using DIC microscopy, the number of cell corpses quantified include early stage apoptotic cells (corpses begin to cellularize) and the middle to late stage of apoptosis (corpses appear as “buttons” after cellularization out of the germline syncytium) . The cell corpse reporter strains used include the CU1546 strain [ced-1p::ced-1::GFP + rol-6(su1006)] and KX89 strain [ced-4(n1162); lim-7::ced-1::GFP + lin-15] to quantify the number of cells going through the process of engulfment , and the WS2170 strain [lim-1p::YFP::act-5 + unc-119(ed3)], to quantify the early stages of apoptosis . The acridine orange (Sigma) staining protocol was conducted as previously described  with the following modification; the adult hermaphrodites were incubated on NGM plates, seeded with OP50 and 500 µl of acridine orange dissolved in M9 for a final concentration of 0.02 mg/ml; animals were placed in the dark for 2 h prior to visualization. To minimize the acridine orange within the intestine, which can interfere with germline visualization, the animals were transferred to OP50 seeded NGM plates for 1 h before analysis.
DIC microscopy analysis of N2 wild-type, cisd-1(tm4993) and ced-1(e1735) L1 larvae, within 1.5 h of hatching, was conducted to quantify the number of persistent cell corpses as previously described . A total of 30 animals from three independent trials were examined. DIC microscopy analysis of N2 wild-type, cisd-1(tm4993) and ced-1(e1735) bean or comma stage embryos was conducted to quantify the number of somatic programmed cell death corpses. The dying cells, which appeared as refractile discs that are morphologically distinct from other cells, were quantified as previously described .
Nomarski microscopy analysis
Microscopy analysis was conducted similarly as previously described . Briefly, nematodes were mounted on a 3% agarose slide containing an anesthetic solution (0.1% tricane, 0.01% levamisole). Animals were examined using a motorized Zeiss Axioscope fluorescent microscope. Images were collected using the AxioVision 4.7.1 software (Zeiss) and processed using ImageJ (NIH) and Adobe Photoshop CC (Adobe Systems Inc.) software.
All data sets are expressed as mean ± standard deviation (SD). Data sets were analyzed for Gaussian distribution using D’Agostino–Pearson Omnibus normality test or Shapiro–Wilk normality test (alpha = 0.05, P > 0.05). If a normality test was passed, a parametric statistical test was performed; if a normality test was not passed then the data were analyzed using a nonparametric statistical test. Statistical tests conducted include: unpaired t-test, ordinary one-way ANOVA followed by a Dunnett’s multiple comparison test, Kruskal–Wallis test followed by a Dunn’s multiple comparisons test or two-way ANOVA followed by a Sidak’s multiple comparisons test. The statistical test for each experiment is as indicated in the figure legends. P-values are reported with each data set. Data were graphed and analyzed using GraphPad Prism 7.0b.
Chang NC, Nguyen M, Germain M, Shore GC. Antagonism of Beclin 1-dependent autophagy by BCL-2 at the endoplasmic reticulum requires NAF-1. EMBO J. 2010;29:606–18.
Chang NC, Nguyen M, Bourdon J, Risse PA, Martin J, Danialou G, et al. Bcl-2-associated autophagy regulator Naf-1 required for maintenance of skeletal muscle. Hum Mol Genet. 2012;21:2277–87.
Leber B, Andrews DW. Closing in on the link between apoptosis and autophagy. F1000 Biol Rep. 2010;2:88.
Maiuri MC, Criollo A, Kroemer G. Crosstalk between apoptosis and autophagy within the Beclin 1 interactome. EMBO J. 2010;29:515–6.
Tamir S, Rotem-Bamberger S, Katz C, Morcos F, Hailey KL, Zuris JA, et al. Integrated strategy reveals the protein interface between cancer targets Bcl-2 and NAF-1. Proc Natl Acad Sci USA. 2014;111:5177–82.
Wiley SE, Murphy AN, Ross SA, van der Geer P, Dixon JE. MitoNEET is an iron-containing outer mitochondrial membrane protein that regulates oxidative capacity. Proc Natl Acad Sci USA. 2007;104:5318–23.
Colca JR, McDonald WG, Waldon DJ, Leone JW, Lull JM, Bannow CA, et al. Identification of a novel mitochondrial protein (“mitoNEET”) cross-linked specifically by a thiazolidinedione photoprobe. Am J Physiol Endocrinol Metab. 2004;286:E252–260.
Paddock ML, Wiley SE, Axelrod HL, Cohen AE, Roy M, Abresch EC, et al. MitoNEET is a uniquely folded 2Fe 2S outer mitochondrial membrane protein stabilized by pioglitazone. Proc Natl Acad Sci USA. 2007;104:14342–7.
Inupakutika MA, Sengupta S, Nechushtai R, Jennings PA, Onuchic JN, Azad RK, et al. Phylogenetic analysis of eukaryotic NEET proteins uncovers a link between a key gene duplication event and the evolution of vertebrates. Sci Rep. 2017;7:42571.
Chen YF, Kao CH, Chen YT, Wang CH, Wu CY, Tsai CY, et al. Cisd2 deficiency drives premature aging and causes mitochondria-mediated defects in mice. Genes Dev. 2009;23:1183–94.
Sohn YS, Tamir S, Song L, Michaeli D, Matouk I, Conlan AR, et al. NAF-1 and mitoNEET are central to human breast cancer proliferation by maintaining mitochondrial homeostasis and promoting tumor growth. Proc Natl Acad Sci USA. 2013;110:14676–81.
Darash-Yahana M, Pozniak Y, Lu M, Sohn YS, Karmi O, Tamir S, et al. Breast cancer tumorigenicity is dependent on high expression levels of NAF-1 and the lability of its Fe-S clusters. Proc Natl Acad Sci USA. 2016;113:10890–5.
Rondinelli M, Novara F, Calcaterra V, Zuffardi O, Genovese S. Wolfram syndrome 2: a novel CISD2 mutation identified in Italian siblings. Acta Diabetol. 2015;52:175–8.
Amr S, Heisey C, Zhang M, Xia XJ, Shows KH, Ajlouni K, et al. A homozygous mutation in a novel zinc-finger protein, ERIS, is responsible for Wolfram syndrome 2. Am J Hum Genet. 2007;81:673–83.
Urano F. Wolfram syndrome: diagnosis, management, and treatment. Curr Diab Rep. 2016;16:6.
Rouzier C, Moore D, Delorme C, Lacas-Gervais S, Ait-El-Mkadem S, Fragaki K, et al. A novel CISD2 mutation associated with a classical Wolfram syndrome phenotype alters Ca2 + homeostasis and ER-mitochondria interactions. Hum Mol Genet. 2017;26:1786.
Danielpur L, Sohn YS, Karmi O, Fogel C, Zinger A, Abu-Libdeh A, et al. GLP-1-RA corrects mitochondrial labile iron accumulation and improves beta-cell function in type 2 Wolfram syndrome. J Clin Endocrinol Metab. 2016;101:3592–9.
al-Sheyyab M, Jarrah N, Younis E, Shennak MM, Hadidi A, Awidi A, et al. Bleeding tendency in Wolfram syndrome: a newly identified feature with phenotype genotype correlation. Eur J Pediatr. 2001;160:243–6.
Mozzillo E, Delvecchio M, Carella M, Grandone E, Palumbo P, Salina A, et al. A novel CISD2 intragenic deletion, optic neuropathy and platelet aggregation defect in Wolfram syndrome type 2. BMC Med Genet. 2014;15:88.
Gartner A, Boag PR, Blackwell TK. Germline survival and apoptosis. WormBook: the online review of C elegans biology. 2008; 1-20.
Conradt B, Wu YC, Xue D. Programmed Cell Death During Caenorhabditis elegans Development. Genetics. 2016;203:1533–62.
Hubbard EJ, Greenstein D. Introduction to the germ line. WormBook: the online review of C elegans biology. 2005; 1-4.
Ye AL, Ragle JM, Conradt B, Bhalla N. Differential regulation of germline apoptosis in response to meiotic checkpoint activation. Genetics. 2014;198:995–1000.
Gumienny TL, Lambie E, Hartwieg E, Horvitz HR, Hengartner MO. Genetic control of programmed cell death in the Caenorhabditis elegans hermaphrodite germline. Development. 1999;126:1011–22.
Hengartner MO, Horvitz HR. Programmed cell death in Caenorhabditis elegans. Curr Opin Genet Dev. 1994;4:581–6.
Ellis HM, Horvitz HR. Genetic control of programmed cell death in the nematode C. elegans. Cell. 1986;44:817–29.
Lee M, Cram EJ. Quantitative analysis of distal tip cell migration in C. elegans. Methods Mol Biol. 2009;571:125–36.
Kelly WG, Fire A. Chromatin silencing and the maintenance of a functional germline in Caenorhabditis elegans. Development. 1998;125:2451–6.
Dickinson DJ, Pani AM, Heppert JK, Higgins CD, Goldstein B. Streamlined genome engineering with a self-excising drug selection cassette. Genetics 2015;4:1035–49.
Holt SH, Darash-Yahana M, Sohn YS, Song L, Karmi O, Tamir S, et al. Activation of apoptosis in NAF-1-deficient human epithelial breast cancer cells. J Cell Sci. 2016;129:155–65.
Cram EJ, Shang H, Schwarzbauer JE. A systematic RNA interference screen reveals a cell migration gene network in C. elegans. J Cell Sci. 2006;119:4811–8.
Wu YC, Horvitz HR. C. elegans phagocytosis and cell-migration protein CED-5 is similar to human DOCK180. Nature. 1998;392:501–4.
Reddien PW, Horvitz HR. CED-2/CrkII and CED-10/Rac control phagocytosis and cell migration in Caenorhabditis elegans. Nat Cell Biol. 2000;2:131–6.
Lant B, Derry WB. Methods for detection and analysis of apoptosis signaling in the C. elegans germline. Methods. 2013;61:174–82.
Kinchen JM, Cabello J, Klingele D, Wong K, Feichtinger R, Schnabel H, et al. Two pathways converge at CED-10 to mediate actin rearrangement and corpse removal in C. elegans. Nature. 2005;434:93–99.
Zhou Z, Hartwieg E, Horvitz HR. CED-1 is a transmembrane receptor that mediates cell corpse engulfment in C. elegans. Cell. 2001;104:43–56.
Kinchen JM, Doukoumetzidis K, Almendinger J, Stergiou L, Tosello-Trampont A, Sifri CD, et al. A pathway for phagosome maturation during engulfment of apoptotic cells. Nat Cell Biol. 2008;10:556–66.
Hengartner MO, Ellis RE, Horvitz HR. Caenorhabditis elegans gene ced-9 protects cells from programmed cell death. Nature. 1992;356:494–9.
Conradt B, Horvitz HR. The C. elegans protein EGL-1 is required for programmed cell death and interacts with the Bcl-2-like protein CED-9. Cell. 1998;93:519–29.
Schumacher B, Schertel C, Wittenburg N, Tuck S, Mitani S, Gartner A, et al. C. elegans ced-13 can promote apoptosis and is induced in response to DNA damage. Cell Death Differ. 2005;12:153–61.
Nehme R, Conradt B. egl-1: a key activator of apoptotic cell death in C. elegans. Oncogene. 2008;27:S30–40.
Karmi O, Holt SH, Song L, Tamir S, Luo Y, Bai F, et al. Interactions between mitoNEET and NAF-1 in cells. PLoS One. 2017;12:e0175796.
Fairlie WD, Perugini MA, Kvansakul M, Chen L, Huang DC, Colman PM. CED-4 forms a 2: 2 heterotetrameric complex with CED-9 until specifically displaced by EGL-1 or CED-13. Cell Death Differ. 2006;13:426–34.
Tamir S, Paddock ML, Darash-Yahana-Baram M, Holt SH, Sohn YS, Agranat L, et al. Structure-function analysis of NEET proteins uncovers their role as key regulators of iron and ROS homeostasis in health and disease. Biochim Biophys Acta. 2015;1853:1294–315.
Kamath RS, Fraser AG, Dong Y, Poulin G, Durbin R, Gotta M, et al. Systematic functional analysis of the Caenorhabditis elegans genome using RNAi. Nature. 2003;421:231–7.
Reddien PW, Horvitz HR. The engulfment process of programmed cell death in Caenorhabditis elegans. Annu Rev Cell Dev Biol. 2004;20:193–221.
Brenner S. The genetics of Caenorhabditis elegans. Genetics. 1974;77:71–94.
Contreras V, Friday AJ, Morrison JK, Hao E, Keiper BD. Cap-independent translation promotes C. elegans germ cell apoptosis through Apaf-1/CED-4 in a caspase-dependent mechanism. PLoS One. 2011;6:e24444.
Yuan J, Horvitz HR. The Caenorhabditis elegans cell death gene ced-4 encodes a novel protein and is expressed during the period of extensive programmed cell death. Development. 1992;116:309–20.
Mitani S. Nematode, an experimental animal in the national BioResource project. Exp Anim. 2009;58:351–6.
Sievers F, Wilm A, Dineen D, Gibson TJ, Karplus K, Li W, et al. Fast, scalable generation of high-quality protein multiple sequence alignments using Clustal Omega. Mol Syst Biol. 2011;7:539.
Berkowitz LA, Knight AL, Caldwell GA, Caldwell KA. Generation of stable transgenic C. elegans using microinjection. J Vis Exp. 2008;17:835.
Kamath RS, Ahringer J. Genome-wide RNAi screening in Caenorhabditis elegans. Methods. 2003;30:313–21.
Mendenhall AR, LaRue B, Padilla PA. Glyceraldehyde-3-phosphate dehydrogenase mediates anoxia response and survival in Caenorhabditis elegans. Genetics. 2006;174:1173–87.
Timmons L, Fire A. Specific interference by ingested dsRNA. Nature. 1998;395:854.
Garcia AM, Ladage ML, Dumesnil DR, Zaman K, Shulaev V, Azad RK, et al. Glucose induces sensitivity to oxygen deprivation and modulates insulin/IGF-1 signaling and lipid biosynthesis in Caenorhabditis elegans. Genetics. 2015;200:167–84.
Ladage ML, King SD, Burks DJ, Quan DL, Garcia AM, Azad RK, et al. Glucose or altered ceramide biosynthesis mediate oxygen deprivation sensitivity through novel pathways revealed by transcriptome analysis in Caenorhabditis elegans. G3 (Bethesda). 2016;6:3149–60.
Hoogewijs D, Houthoofd K, Matthijssens F, Vandesompele J, Vanfleteren JR. Selection and validation of a set of reliable reference genes for quantitative sod gene expression analysis in C. elegans. BMC Mol Biol. 2008;9:9.
Schwartz HT. A protocol describing pharynx counts and a review of other assays of apoptotic cell death in the nematode worm Caenorhabditis elegans. Nat Protoc. 2007;2:705–14.
Mendenhall AR, LeBlanc MG, Mohan DP, Padilla PA. Reduction in ovulation or male sex phenotype increases long-term anoxia survival in a daf-16-independent manner in Caenorhabditis elegans. Physiol Genom. 2009;36:167–78.
Lints R, Hall DH. Reproductive system, germ line. WormAtlas 2009. Available from: http://www.wormatlas.org/hermaphrodite/germline/Germframeset.html.
This work is supported by a grant from the NSF IOS (1557787) to P.A.P. (PI) and R.M. (CoPI). We thank Ed Dzialowski and members of the Padilla lab for input. We thank WormBase, supported by grant U41 HG002223 from the National Human Genome Research Institute at the National Institutes of Health (NIH), for providing valuable genomic database information. We thank the Caenorhabditis elegans Genetics Center, which is funded by NIH Office of Research Infrastructure Programs (P40 OD010440), and the National Bioresource Project for the Nematode, Tokyo, Japan, for strains.
Conflict of interest
The authors declare that they have no conflict of interest.
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King, S.D., Gray, C.F., Song, L. et al. The cisd gene family regulates physiological germline apoptosis through ced-13 and the canonical cell death pathway in Caenorhabditis elegans. Cell Death Differ 26, 162–178 (2019). https://doi.org/10.1038/s41418-018-0108-5
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