Tfam Knockdown Results in Reduction of mtDNA Copy Number, OXPHOS Deficiency and Abnormalities in Zebrafish Embryos

Introduction

Mitochondria are responsible for producing the majority of cellular energy in the form of ATP. Depending on the tissue type and energy requirement, a cell can contain up to thousands of mitochondria, each having multiple copies of mitochondrial DNA (mtDNA). Of all cell-types, mtDNA copy numbers are the highest in oocytes, ranging between 100,000 and 400,000 copies in mammals, such as rodents, cows and humans, and up to 16.5 million copies in zebrafish (Otten and Smeets, 2015). The high mtDNA copy number in oocytes is established by an initial reduction during embryogenesis, called the mitochondrial bottleneck, followed by clonal expansion of the mtDNA during oogenesis appears to be important for successful fertilization and embryogenesis (Santos et al., 2006). In mice, the oocyte mtDNA copy number should be sufficient for normal development until implantation at day 4, and it has been demonstrated that oocytes with less than 50,000 mtDNA copies fail to resume development after implantation (Ebert et al., 1988; Wai et al., 2010). This negative correlation between mtDNA copy number and developmental competence of embryos has also been suggested for human oocytes (Yamamoto et al., 2010).

Mitochondrial transcription factor A (TFAM), a protein of the high mobility group box-family, is a key activator of mtDNA replication and transcription (Parisi et al., 1993) and is crucial for the regulation of mtDNA copy number (Larsson et al., 1998). A direct relation between the mtDNA copy number and the total TFAM protein level has been demonstrated in mice embryos with a heterozygous or homozygous disruption of the Tfam gene (Ekstrand et al., 2004). Homozygous TFAM knockout (KO) mouse embryos displayed a strong mtDNA depletion with severely reduced functioning of the electron transport chain (ETC) and died after gastrulation and implantation, while heterozygous KO TFAM mice had moderately reduced mtDNA levels and respiratory chain deficiency, which was strongest in the developing heart (Larsson et al., 1998). These studies demonstrated the importance of a sufficient mtDNA copy number during oogenesis and embryogenesis, but the mechanism by which a reduced mtDNA copy number affects embryogenesis is currently unknown.

Studying embryonic development in zebrafish overcomes ethical and practical obstacles associated with the use of human or mouse embryos. Zebrafish are vertebrates, >70% of human genes have at least one zebrafish orthologue, and the major tissues and organs are the same. Zebrafish are transparent during early development and have a high number of offspring. Organs develop within 5 days post fertilization and gene knockdown during early embryogenesis can be performed by injection of morpholino antisense oligonucleotides (MOs) (Pauli et al., 2015). Previously, we showed that the mitochondrial bottleneck during early development is highly conserved between zebrafish and mammals (Otten et al., 2016). In addition, the zebrafish Tfam protein is functionally homologous to its human counterpart and is expressed ubiquitously from the earliest stages of development (Artuso et al., 2012). In this study, we performed tfam knockdown during zebrafish embryogenesis in order to reduce the mtDNA copy number during early development. In this way, we created an animal model with a tuneable mtDNA bottleneck, which allows us to assess the effect of differences in mtDNA copy number on OXPHOS function and embryonic development and to determine the underlying mechanisms.

Materials and Methods

Zebrafish Maintenance and Procedures

Zebrafish (Danio rerio) were housed and raised in the zebrafish facility of the University of Liège as described before (Larbuisson et al., 2013). To retrieve eggs, wild-type adult male and female zebrafish were separated within the same breeding tank by a plastic divider the day before breeding. This separation was removed the next day after the light was turned on in order to allow natural mating and eggs were collected after spawning. Eggs were collected in Petri dishes containing 1× E3 medium for zebrafish at 28°C (580 mg/l NaCl, 27 mg/l KCl, 97 mg/l CaCl₂⋅2H₂O, 163 mg/l MgCl₂⋅6H₂O and 0.0001% methylene blue (Sigma-Aldrich), pH 7.2) (Larbuisson et al., 2013). Embryos were microscopically staged according to the embryonic development as described before (Kimmel et al., 1995). Unless stated otherwise, all reagents used in this study were obtained from Thermo Fisher Scientific.

Tfam Knockdown Experiments

Antisense morpholino oligonucleotides (MO) were purchased from Gene Tools and micro-injected into one or two-cell stage embryos. A splice modifying MO was used, targeting the boundary of exon 2 and intron 2–3 of the zebrafish tfam gene (Ensemble: ENSDART00000092009, tfam splice-MO: 5′-CGGCAGATGGAAATTTACCAGGATT-3 ′). For controlling the effect of the MO injection, an equal concentration of a standard control-morpholino (Ctrl-MO: 5′-CCTCTTACCTCAGTTACAATTTATA-3′) was used in separate embryos of the same batch during each experiment. All MOs were dissolved in 1× Danieau buffer (58 mM NaCl, 0.7 mM KCl, 0.4 mM MgSO₄, 0.6 mM Ca(NO₃)₂, and 5.0 mM HEPES pH 7.6) and 0.5% rhodamine dextran (Thermo Fisher) was added to the MO solution upon injection. At 1 hpf, 1 nl was injected into each embryo using microinjection (Bill et al., 2009). The next day, distribution of the rhodamine dextran dye was checked using fluorescence stereomicroscopy to verify proper injections. Only those embryos in which the rhodamine dextran dye was visible were used for follow-up investigations.

Quantitative and Qualitative Analysis of Tfam RNA

Total RNA of 2–4 dpf zebrafish embryos was extracted using Trizol reagent and purified using the RNeasy Mini Kit (Qiagen), according to manufacturer’s instructions. cDNA synthesis was performed with 500 ng RNA in the presence of first strand buffer, 0.75 μg oligo-dT, 0.75 μg random hexamer-primer, 50 nmol dNTPs (GE Healthcare Life Sciences), 1 U RNAse inhibitor (RNAsin, Promega) and 5 U reverse transcriptase for 60′ at 42°C, followed by 5′ at 95°C. The effect on tfam splicing was assessed using RT-PCR amplification of 25 ng cDNA in a PCR mix contained under standard conditions, using 0.6 μM forward primer, 0.6 μM reverse primer (Supplementary Table S1). PCR conditions were 5′ denaturation at 94°C, 35 cycles of 1′ at 94°C, 1′ at 58°C and 1,5′ at 72°C, followed by 7′ at 72°C. The PCR product was sequenced by conventional Sanger sequencing. tfam gene expression was quantified by comparing the RNA expression ratio of Tfam RNA to 18S RNA. Per reaction, 2.5 ng cDNA was amplified in a 10 μl reaction containing 1× Sensimix Sybr Hi-Rox reagents (Bioline) and 375 nM of both forward and reverse primer (Supplementary Table S1). Real-time PCR was performed on an ABI7900HT using the following settings: 10′ 95°C, 40 cycles of 15” 95°C and 1′ 60°C. The statistical analysis was performed by a Student’s t-test. p-values < 0.05 were considered significant.

Quantification of mtDNA Copy Number

To determine mtDNA copy number, embryos were individually collected in sterile tubes and directly frozen without water. For DNA isolation, embryos were thawed and lysed for 4 h at 55°C in lysis buffer containing 75 mM NaCl, 50 mM EDTA, 20 mM HEPES, 0.4% SDS and 200 μg proteinase K (Sigma) while vortexing repeatedly. DNA precipitation was performed overnight at −20°C after adding 420 μl isopropanol. Following centrifugation, the DNA pellet was washed with 70% ethanol and dissolved in Tris-EDTA buffer. The relative mtDNA abundance was quantified by measuring the steady-state amount of mitochondrial ND1 and nuclear B2M. Per reaction, 20 ng DNA was used in a 10 μl reaction containing 1× Sensimix Sybr Hi-Rox reagents (Bioline) and 375 nM of both forward and reverse primer (Supplementary Table S1). Real-time quantification was performed on an ABI7900HT as described before. Statistical analysis was carried out using one-way analysis of variance (ANOVA) followed by the Bonferroni multiple comparisons test. P-values < 0.05 were considered significant.

Imaging of Zebrafish Embryos

Zebrafish embryos were fixed at 4°C with paraformaldehyde for 4 h and standard paraffin serial sections of 4 μm thickness were prepared for immunostaining and hematoxylin-eosin (HE)-staining. Immunohistochemistry was performed following a microwave heat-induced antigen retrieval step for four times 5′ at 650 Watt (in Tris-EDTA, pH = 9.0) and was analyzed with the Dako REALTM EnVisionTM Detection System, Peroxidase/DAB, Rabbit/Mouse, using a Dako automated immunostaining instrument and protocols according to the manufacturer (Agilent, Santa Clara). Antibodies and conditions used are listed in Supplementary Table S1. HE-staining was performed to reveal the underlying embryonic structures. Paraffin slides were embedded in Entellan (Merck) and protected by cover slips (Knittel Glass). Microscopic images were taken by using the Nikon Eclipse E80 Imaging System (Nikon) at different magnifications. The orientation of fish was determined according to the Zebrafish Bio-Atlas¹ (Cheng, 2004, 8 August).

Oxygen Consumption Rate

At 4 dpf, chorion-free living fish embryos with a heartbeat and active swimming behavior upon touching were selected and collected individually. The oxygen consumption rate (OCR) (pmol/minute) was measured every minute for 15 min in a Seahorse XF24 system (Agilent/Seahorse Biosciences), according to the islet protocol of the manufacturer with 2 fish per well of a 24-well plate. Five minutes after starting the assay, 80 μM of Oligomycin (Sigma-Aldrich) was added and 60 μM for Antimycin & Rotenone (Sigma-Aldrich) in the injecting assay medium (1× E3 medium) was added 10 min after start. The OCR level at basal respiration (pmol/min) was calculated using the OCR values at the start respiration level (time-point 5 min) minus antimycin/rotenone (AMA) level at time-point 10 min. Maximal ATP production (pmol/min) was determined as start respiration level minus oligomycin (OMY) level at time-point 15 min. The statistical analysis was performed by a Student’s t-test. p-values < 0.05 were considered significant.

Gene Expression and Pathway Analysis

For gene expression studies, tfam splice-MO and control-MO injected embryos and non-injected control embryos at 4 dpf, were individually collected in sterile tubes. Selection criteria were the same as for the OCR measurements. RNA from single embryos was isolated using the MagMax-96 for microarray kit (Ambion) and 200 ng RNA was labeled (Cyanine 3-CTP and Cyanine 5-CTP), fragmented and hybridized using the Low Input Quick Amp Labeling Kit, Two-colour (Ambion), according to manufacturer’s instructions. After labeling, amplified cRNA samples were purified using the RNeasy Mini kit (Qiagen) and Cyanine 3 and Cyanine 5 dye concentration, RNA absorbance ratio (260/280 nm) and cRNA concentration were quantified using the nanodrop 2000C (Thermo Fisher Scientific). Only samples with a yield > 0.825 μg and a specific dye activity >6.0 pmol/μg were used for fragmentation and hybridization. For fragmentation, 825 ng labeled cRNA was used and the final volume was adjusted to 41.8 μl with RNAse-free water, followed by the hybridization procedure, as described by the manufacturer (Ambion). Dye-swap hybridizations (2+2) were performed on microarray slides (4×44K zebrafish V3, Agilent) using gasket slides and a hybridization chamber and incubated for 17 h at 65°C and 10 rpm in the hybridization oven (Agilent Technologies). Slides were washed with Triton X-102, freshly added to the Wash Buffers. Microarray slides were scanned using a DNA Microarray scanner with Surescan High-Resolution Technology (Model 2565CA, Agilent). All microarray data is deposited in the GEO database, accession GSE146696.

The arrays contained 45,220 probes. Each probe identifier was transformed to Ensembl gene IDs (ENSDARG). This resulted in 36,156 probes containing a non-empty transcript ID of which 19,459 were unique transcripts and kept for the analysis. All transcripts were analyzed using a multivariate Gaussian linear regression MVN(μ, Σ) where μ is the mean, Σ is the covariance matrix $\left(\begin{array}{cccc}{\sigma }^2+\delta & \delta & \cdots & \delta \\ \delta & \ddots & \ddots & ⋮\\ ⋮& \ddots & \ddots & \delta \\ \delta & \cdots & \delta & {\sigma }^2+\delta \end{array}\right),{\sigma }^2$ is the variance, and δ is both the extra component of variance across subjects and the common covariance among responses on the same subject) including slide differences (Slide), dye swap (Dye), background level (Bg), injection (Inj), and a random effect. The inference criterion used for comparing the models is their ability to predict the observed data, i.e., models are compared directly through their minimized minus log-likelihood. When the numbers of parameters in models differ, they are penalized by adding the number of estimated parameters, a form of the Akaike information criterion (Akaike, 1973). For each transcript, a model containing the relevant covariates mentioned above (E(y) = Slide + Dye + Bg + Inj) was fitted in order to obtain a reference AIC. Then a model containing the treatment group (Trt) was fitted (E(y) = Slide + Dye + Bg + Inj + Inj:Trt). The transcript under consideration was found to be differentially expressed if the AIC of this second model decreased compared to the model not containing the treatment. These statistical analysis were performed using the freely available program R (Ihaka, 1996) and the publicly available libraries “rmutil” and “growth” (Lindsey, 1999). An unbiased Gene-ontology analysis and visualization of microarray data on biological pathways was performed using PANTHER (Protein Analysis THrough Evolutionary Relationships) with the D. rerio (Dr_Derby_Ensembl_80) gene product/protein database (Thomas et al., 2003; Mi et al., 2017). Differentially expressed genes (DEGs) were mapped to unique Entrez Gene IDs and to Gene Ontology (GO) classes, using the PANTHER Overrepresentation Test (Released 2018-02-03) enrichment method of PANTHER version 13.1.

Results

Tfam Knockdown Results in Decreased mtDNA Content and Mitochondrial ATP Production

To establish decreased mtDNA copy number, we microinjected an antisense splice-MO targeting tfam-mRNA in zebrafish embryos. Using RT-PCR and Sanger sequencing of cDNA from tfam splice-MO-injected 4 dpf embryos (n = 6/group), we showed that the tfam splice-MO causes a 128 base-pair deletion of exon 2 (c.84_211del), predicted to cause a frameshift and a premature stop codon (p.(Cys29Hisfs^∗36)) (Figure 1A and Supplementary Figure S1). Quantitative PCR analysis of tfam exon 5 and exon 6–7 showed, respectively, 59 ± 2% and 60 ± 5% decrease in expression in tfam splice-MO injected embryos at day 4 (mean ± SD, n = 6/group). qPCR analysis of tfam exon 2 expression showed a reduction of 80 ± 3% at day 4 in zebrafish (n = 6/group) injected with 2 ng tfam splice-MO compared to the Ctrl-MO (Supplementary Figure S2). This indicates that ∼60% of tfam RNA is subjected to nonsense-mediated decay and that of the residual ∼40% tfam RNA, only half is exon 2-containing wild-type RNA (only 20% of normal tfam amount). Next, we assessed the mtDNA copy number in non-injected, Ctrl-MO injected and tfam splice-MO injected embryos (n = 20 in each 2 ng group, and n = 16 in each 4 ng group). At 4 dpf, a significant, 42 ± 17% (mean ± SD) decrease in the mtDNA copy number was observed in embryos injected with either 2 ng or 4 ng tfam splice-MO (Figure 1B). In contrast, no significant differences in mtDNA copy number were apparent between groups at 2 dpf (Supplementary Figure S3). To assess if decreased mtDNA copy number also affected mitochondrial capacity, we measured the OCR at 4 dpf. As shown in Figure 1C, both the OCR of the basal respiration and the ATP production were significantly decreased in the 2 ng tfam splice-MO treated zebrafish (n = 10) compared with the 2 ng control-MO treated group (n = 9) (p < 0.05) by respectively, 40 ± 25 and 50 ± 22% (mean ± SD).

FIGURE 1

Figure 1. Knockdown of TFAM in zebrafish embryos. Zebrafish embryos injected with indicated amount of either Control-morpholino (Ctrl-MO) or tfam splice-morpholino tfam splice-MO at 1 hpf and analyzed at 4 dpf. (A) tfam splice-morpholino (MO) at the 3′ splice site of exon 2 causes deletion of exon 2, which predicts a frame-shift and premature stop codon (p.(Cys29Hisfs*36)) (figure is not on scale). (B) The relative copy number assessed by mitochondrial ND1/nuclear B2M ratio. Data are normalized to the NIC embryos (n = 7). Bars indicate mean values with SD, n = 20 per 2 ng injected condition and n = 16 per 4 ng injected condition. P-values are calculated using ANOVA followed by Bonferroni’s Multiple Comparison Test to assess copy number, *P-value < 0.05, **P-value < 0.01. (C) The oxygen consumption rate (OCR) measured by Seahorse XF24 in order to assess basal respiration and maximal ATP production capacity at 4 dpf using 2 ng MO. The statistical analysis was performed by using a student t-test (P < 0.05), n = 10 per tfam splice-MO condition and n = 9 per Ctrl-MO condition.

Decreased mtDNA Copy Number Causes Brain, Eye, Heart, and Muscle Abnormalities

At 4 dpf, morphant embryos displayed morphological abnormalities compared to control embryos. The macroscopic phenotype included overall oedema, curved tails, necrotized yolk sacs and small eyes (Supplementary Figure S4). Fish injected with 4 ng tfam splice-MO were more severely affected than 2 ng tfam splice-MO (n = 100 injected per condition), as they had a higher count for oedema, curved tails, necrotized yolk sac, small eyes, and developmental delay. The percentage of dead embryos was <1% when injecting 2 or 4 ng of tfam MO-injections at 4 dpf (Supplementary Figure S4). In contrast, injection of 6 ng of tfam splice-MO showed >70% of embryonic lethality due to severe developmental complications. Macroscopic inspection of tfam splice-MO injected embryos showed that all observed pathologies manifested at 3 or 4 dpf, whereas development was apparently normal at 2 dpf. These morphological changes parallel the decrease in mtDNA copy number that is observed at 4 dpf, but not at 2 dpf (Figure 1B and Supplementary Figure S3). Since the decrease in mtDNA content was comparable with 4 ng tfam splice-MO, the dosage of 2 ng tfam splice-MO was used in all following experiments, reducing the risk of non-specific observations.

Microscopic evaluation of zebrafish (n = 13 per condition) with reduced mtDNA copy number using 2 ng tfam splice-MO showed impaired development compared to control embryos (Figure 2). Brain size was decreased with no or less well-developed cerebellum (Figure 2B), and the eyes were smaller and the different layers were less-well organized compared to controls (Figure 2D). Also, the organization of the myotomic area was less compact with the skeletal muscle fibres being thinner and disorganized (Figure 2F). Finally, morphant fish displayed marked pericardial oedema, alongside with a dilated non-looped heart (Figure 2H).

FIGURE 2

Figure 2. Microscopy of zebrafish embryos following TFAM knockdown. (A–H) Microscopic analysis following serial HE-staining of zebrafish embryos at 4 dpf, which were injected at 1 hpf with either 2 ng tfam splice-MO (B–E) or 2 ng Ctrl-MO, (A,C,E,G) n = 13 each condition. (B) The cerebellum was missing in the phenotype or a delayed development of this cerebellum in these fish. (D) The eyes were smaller and the eye layers were less developed. (F) A muscle phenotype was clearly visible in the dorsal fin, especially in the myotomic area, which was less compact in these somatic muscles. (H) The fish displayed a marked pericardial oedema (red arrow). They did not develop a normally looped heart as in Ctrl-MO (G), but the hearts were dilated in the phenotypes (H).

Genes and Pathways Altered by Tfam Knockdown

To characterize the underlying pathogenic processes due to tfam knockdown and subsequent decrease in mtDNA copy number, we compared global gene expression profiles at 4 dpf of zebrafish injected with 2 ng of either tfam splice-MO (n = 12) or Ctrl-MO (n = 12). A group of non-injected control zebrafish was also included (n = 9) to control for the injection effect in the microarray analysis and allow identification of transcripts altered in the tfam splice-MO zebrafish compared with the Ctrl-MO zebrafish. A total of 19,459 transcripts were present on the array (Supplementary Table S2), of which 16,631 (85.5%) had a signal intensity higher than twice the background signal in both conditions or a signal that was at least three times higher than the background signal in either the group of tfam splice-MO zebrafish or the group of Ctrl-MO zebrafish. Of these, 3,158 transcripts (19.3%) were differentially expressed between the two groups with a fold change (FC) >50%. Expression of 2,063 transcripts (64.3%) was increased (FC ≥ 1.50), while expression of 1,145 transcripts (35.7%) was decreased in the tfam splice-MO injected embryos (FC ≤ 0.67). In order to identify significantly altered pathways by using gene ontology analysis, Protein ANalysis THrough Evolutionary Relationships (PANTHER) was used. The microarray contained 19,459 transcripts, of which 17,395 could be annotated (89.4%) and were included in the PANTHER analysis. A total of 18 significantly enriched GO biological processes (FDR < 0.05) were identified and these were manually grouped into five groups including the underlying GO terms, namely: tRNA processing, ribosome biogenesis, RNA surveillance and catabolism, drug metabolism, and visual perception (Table 1 and Supplementary Table S4). As the RNA-related processes differ for nuclear and mtDNA genes and for that reason should not be considered as one group, we also listed the mitochondria-related processes, characterized by mitochondria-related GO terms (Table 2 and Supplementary Table S5). Most of the mitochondria related GO terms were small, comprising less than 50 measured genes, but sufficient number of genes were interrogated to conclude that these processes were not significantly enriched by the mtDNA reduction. However, as expression of mtDNA encoded proteins, which is regulated by TFAM, was not covered in a GO term, we checked the expression of the 8 mtDNA protein encoding genes manually. The 8 mtDNA proteins encoding transcripts of the H-strand were significantly decreased, whereas the single L-strand transcript was unaltered (Supplementary Table S3). The remainder four protein encoding transcripts of the H-strand were not present on the array (atp6, atp8, cox 3, and cytb).

TABLE 1

Table 1. Significantly altered GO biological process terms.

TABLE 2

Table 2. Mitochondria-related GO biological processes.

Discussion

A high mtDNA copy number is critical for normal embryonic development. A key regulator of the mtDNA copy number is TFAM, as TFAM initiates mtDNA replication by its capability to wrap, bend and unwind the mtDNA (Ekstrand et al., 2004), a function conserved in zebrafish (Howe et al., 2013). In order to study the effect of a decreased mtDNA copy number during zebrafish embryonic development, we performed tfam knock-down using a splice-morpholino (MO). We demonstrated that the tfam splice-MO induced skipping of exon 2, leading to a frameshift and a premature stop codon (p.(Cys29Hisfs^∗36)) (Figure 1A) and to nonsense mediated decay. RNA expression of normal tfam is reduced to 20% of control values. At 3 and 4 dpf, morphant zebrafish have a decreased mtDNA copy number and are less well developed. This correlates with the previous observations that in wild-type zebrafish larvae an increase in mtDNA copy number only becomes apparent between 2 and 3 dpf (Otten et al., 2016) indicating that, in the absence of mtDNA replication, mtDNA copy number and OXPHOS capacity becomes critically low at 3–4 dpf, as an increase is required for embryonic tissue differentiation and organogenesis. This is a critical phase of development, when there is a high energy demand and a metabolic switch from glycolysis to OXPHOS takes place (Hance et al., 2005; Stackley et al., 2011). This necessity is illustrated by the aberrant eye and muscle development, pericardial oedema and reduced brain size that were observed in morphant zebrafish (Figure 2). The heart and the brain are the first organs to develop (Glickman and Yelon, 2002) and therefore the first to be affected by OXPHOS defects. Moreover, as in a normal heart >30% of the cardiac muscle volume is occupied by mitochondria, the deficit of mtDNA (and subsequently mitochondria) also hampers proper alignment of the muscle fibers in the developing heart, creating structural problems as well (Ventura-Clapier et al., 2011). In homozygous Tfam KO mice, OXPHOS was abolished due to a severe mtDNA depletion, causing a complete failure of organogenesis and embryonic death (Larsson et al., 1998). Heterozygous KO mice were viable, but showed an OXPHOS deficiency in the developing heart and a dilated cardiomyopathy and conduction block later in life (Larsson et al., 1998; Powell et al., 2015). The severity of our model seems to fit somewhere in between, as wild-type tfam levels are around 20% of control level at the day of analysis. Noticeably, MOs establish only a transient knockdown, which is not the case for a homozygous or heterozygous knockout of the gene, prohibiting a proper comparison later in life.

In order to unravel the biological processes that were altered, we performed global gene expression profiling and subsequent gene ontology (GO) analysis (Table 1 and Figure 3). Despite the observed reduction in OXPHOS function, the gene ontology term comprising mitochondrial respiratory chain components was not significantly changed, neither were critical mitochondrial processes (Table 2). However, gene expression was decreased of 8 out of the 9 mtDNA protein encoding transcripts, all encoded by the H-strand, whereas the one transcript on the L-strand was unaltered. This most likely this reflects a switch or preferable transcription from the Light-Strand Promoter (LSP) that is induced by low amounts of tfam and which also primes H-strand replication (Shutt et al., 2011), but which in our case fails to increase mtDNA copy number due to the persisting lack of tfam.

FIGURE 3

Figure 3. Schematic overview of alterations in tfam splice-MO zebrafish at 4dpf. The arrow indicates if a process is upregulated (green) or down-regulated (red). Altered gene expression processes and genes are shown in italic. The mitochondrial DNA figure is adapted from Amorim et al. (2019).

The GO term drug catabolism was significantly changed, comprising several downregulated genes linked to mitochondrial function, including embryonic hemoglobin production. As haem is produced by mitochondria (Wagener et al., 2003), this could be explained by the decreased amount of mtDNA and subsequently mitochondria at the onset of definitive haematopoiesis, initiating between 1 to 2 dpf (Murayama et al., 2006; Bertrand et al., 2007; Zhang and Rodaway, 2007; Zhang and Hamza, 2018). Obviously, deficiencies in haematopoiesis during development might have downstream effects as well. Other mitochondria-related genes of this GO term were decreased, such as oxct1a, oxct1b, members of cyp450 family 2 and gpx1a, which are related to the metabolism of fatty acids and ketone bodies, exogenous drug catabolism and hydrogen peroxide degradation in the mitochondria. The decrease in mtDNA copy number and subsequent mitochondrial dysfunction appears to result in enrichment of GO terms related to rRNA synthesis, ncRNA processing, and ribosomal assembly (Table 1), and the vast majority of genes in these GO terms were upregulated (Supplementary Table S4). In addition, the GO term tRNA processing was also significantly enriched. In general, expression of genes belonging to these GO terms is increased, including a number of genes that are linked to mitochondrial function, like mto1 (1.64), trmt10c (1.55), and elac2 (1.61) (Haack et al., 2013; Metodiev et al., 2016; Fakruddin et al., 2018). Increased tRNA synthesis was also observed by Torrent et al. (2018) upon applying diverse stress conditions to Saccharomyces cerevisiae, demonstrating the regulation of tRNA abundance upon cellular stress. However, future research is needed to identify if the observed activation nucleolar processes is caused by mitochondrial stress or is a reaction to compensate for the reduction in mitochondrial transcripts. The resulting disbalance between mitochondrial transcripts and proteins, and nuclear encoded proteins that migrate into the mitochondria might be a factors as well. Also, gene expression of 8 out of 9 exosome components, belonging to GO term ribosomal biogenesis, were significantly upregulated in tfam splice-MO zebrafish. Like increased rRNA and tRNA expression, upregulation of the exosome components seems to be a compensatory or stress-induced mechanism, as exosomes contain and shuttle mRNA, and are important in intercellular communication and developmental patterning (Wan et al., 2012; Boczonadi et al., 2014; McGough and Vincent, 2016). Future assessment of the zebrafish exosome composition is needed to provide further insight into this novel mechanism by which decreased mtDNA copy number affects exosome signalling and composition.

Since clear morphological abnormalities were apparent in tfam splice-MO zebrafish at 4 dpf (Figure 2), the nucleolar activation upon mitochondrial deficiency was obviously insufficient to compensate. At gene expression level in tfam splice-MO zebrafish at 4 dpf, GO terms related to vision and sensitivity to light were significantly changed. Retinal development is critical between 32 and 74 hpf and normally largely completed at 4 dpf (Richardson et al., 2017). This window coincides with the decrease in mtDNA copy number in tfam splice-MO zebrafish, explaining the down-regulation observed. These extremely down-regulated eye genes are mainly involved in processes related to response to light stimulus (Supplementary Table S4), like pde6c (0.05) and gnat2 (0.09). Zebrafish mutants of these genes respectively cause retinal and retinal pigment epithelial disease and cone-rod dystrophy (Brockerhoff et al., 2003; Richardson et al., 2017). Additional down-regulated opsins genes related to the photoreceptor function are listed in our zebrafish data (Supplementary Table S4). The lack of significant changes in pathways linked to cardiac, muscle or brain development, suggests that although pathology clearly manifested, we are still observing the processes preceding the pathology and not those resulting from it in the pathway analysis. In addition to defective eye development, a number of temporally expressed developmental genes are downregulated in tfam splice-MO zebrafish at 4 dpf, such as chitinase (Chia) 1, 2, 3 and 4. Expression of chia.1, chia.2 and chia.3, which belong to the GO term drug metabolism, normally drastically increases at 4 and 5 dpf, while chia.4 is more stably expressed. Chitinases are suggested to play a role in early embryo immunity and chitinase inhibition has been shown to cause development disruption in zebrafish, characterized by hampered trunk and tail formation (Semino and Allende, 2000).

In conclusion, inhibition of tfam expression during early zebrafish development leads to a decrease in mtDNA copy number, OXPHOS capacity, and mtDNA encoded transcripts and haem production, affecting the oxygen supply in the developing embryo. This triggers a compensation mechanism or stress response in the nucleoli at the level of rRNA and tRNA biogenesis and translation initiation, but this compensation mechanism falls short, as pathology emerges (Figure 3). The results of this study in zebrafish are comparable to other animal models, thereby validating our model, but they also take it a step further due to the clear advantages of the zebrafish model, being a high number of offspring, a rapid development and an optical clarity during development combined with easy genetic interventions. Being able to tune the mtDNA content, we can now manipulate the mtDNA bottleneck and study in sufficient numbers the effects on processes, like organogenesis, fertility and mtDNA mutation rate.

Data Availability Statement

All microarray data is deposited in the GEO database, accession GSE146696.

Ethics Statement

The animal study was reviewed and approved by the Committee of Animal Research of the University of Liège.

Author Contributions

FT and HS designed and supervised the project. AO and RK designed, performed most of the experiments, and coordinated collaborations with PL, MG, HP-S, and MM. PL designed, assigned, and supplied the transcriptomic computational analysis. RK, FT, and HS determined PANTHER pathway gene-expression analysis on transcriptomic data. AO and RK performed the Tfam knockdown experiments as quantitative and qualitative analysis, imaging embryos, oxygen consumption rate measurements. MG assisted on the design and scientific input on the manuscript. HP-S and MM assisted on the design and scientific input in the manuscript and were coordinating the housing and injections of the zebrafish embryos. All authors contributed to the ideas to the project.

Funding

MM is a “Maître de Recherche,” supported by the “Fonds National pour la Recherche Scientifique” (FNRS). This work was further supported by the Interreg IV program of the European Council (the Alma in Silico project to MM and HS) and the European Research Area Network for Research Programmes on Rare Diseases 2 project GENOMIT (grant R 50.02.12F to MM). Part of this work has been made possible with the support of the Dutch Province of Limburg (MG and HS) and the Research School GROW (AO, PL, and HS).

Conflict of Interest

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Acknowledgments

The authors would like to acknowledge Jo M. Vanoevelen (MUMC+, Maastricht), Ellen EH Lambrichs (MUMC+, Maastricht), Sabina J. V. Vanherle (MUMC+, Maastricht), and Levi GK Wackers (Maastricht University, Maastricht) for their technical laboratory skills and practical contribution to this study. This manuscript has been released as a Pre-Print at BioRxiv 843318v1 (Otten et al., 2019).

Supplementary Material

The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fcell.2020.00381/full#supplementary-material

Footnotes

1. ^ http://bio-atlas.psu.edu

References

Akaike, H. (1973). “Information theory and an extension of the maximum likelihood principle,” in Proceedings of the Second International Symposium on Inference Theory, eds B. N. Petrov and F. Csàki (Budapest: Akadémiai Kiadó), 267–281.

Google Scholar

Amorim, A., Fernandes, T., and Taveira, N. (2019). Mitochondrial DNA in human identification: a review. PeerJ. 7:e7314. doi: 10.7717/peerj.7314

PubMed Abstract | CrossRef Full Text | Google Scholar

Artuso, L., Romano, A., Verri, T., Domenichini, A., Argenton, F., Santorelli, F. M., et al. (2012). Mitochondrial DNA metabolism in early development of zebrafish (Danio rerio). Biochim. Biophys. Acta 1817, 1002–1011. doi: 10.1016/j.bbabio.2012.03.019

PubMed Abstract | CrossRef Full Text | Google Scholar

Bertrand, J. Y., Kim, A. D., Violette, E. P., Stachura, D. L., Cisson, J. L., and Traver, D. (2007). Definitive hematopoiesis initiates through a committed erythromyeloid progenitor in the zebrafish embryo. Development 134, 4147–4156. doi: 10.1242/dev.012385

PubMed Abstract | CrossRef Full Text | Google Scholar

Bill, B. R., Petzold, A. M., Clark, K. J., Schimmenti, L. A., and Ekker, S. C. (2009). A primer for morpholino use in zebrafish. Zebrafish 6, 69–77. doi: 10.1089/zeb.2008.0555

PubMed Abstract | CrossRef Full Text | Google Scholar

Boczonadi, V., Muller, J. S., Pyle, A., Munkley, J., Dor, T., Quartararo, J., et al. (2014). EXOSC8 mutations alter mRNA metabolism and cause hypomyelination with spinal muscular atrophy and cerebellar hypoplasia. Nat. Commun. 5:4287. doi: 10.1038/ncomms5287

PubMed Abstract | CrossRef Full Text | Google Scholar

Brockerhoff, S. E., Rieke, F., Matthews, H. R., Taylor, M. R., Kennedy, B., Ankoudinova, I., et al. (2003). Light stimulates a transducin-independent increase of cytoplasmic Ca2+ and suppression of current in cones from the zebrafish mutant nof. J. Neurosci. 23, 470–480. doi: 10.1523/jneurosci.23-02-00470.2003

PubMed Abstract | CrossRef Full Text | Google Scholar

Cheng, K. C. (2004). A life-span atlas for the zebrafish. Zebrafish 1:69. doi: 10.1089/zeb.2004.1.69

PubMed Abstract | CrossRef Full Text | Google Scholar

Ebert, K. M., Liem, H., and Hecht, N. B. (1988). Mitochondrial DNA in the mouse preimplantation embryo. J. Reprod. Fertil. 82, 145–149. doi: 10.1530/jrf.0.0820145

PubMed Abstract | CrossRef Full Text | Google Scholar

Ekstrand, M. I., Falkenberg, M., Rantanen, A., Park, C. B., Gaspari, M., Hultenby, K., et al. (2004). Mitochondrial transcription factor A regulates mtDNA copy number in mammals. Hum. Mol. Genet. 13, 935–944. doi: 10.1093/hmg/ddh109

PubMed Abstract | CrossRef Full Text | Google Scholar

Fakruddin, M., Wei, F. Y., Suzuki, T., Asano, K., Kaieda, T., Omori, A., et al. (2018). Defective mitochondrial tRNA taurine modification activates global proteostress and leads to mitochondrial disease. Cell Rep. 22, 482–496. doi: 10.1016/j.celrep.2017.12.051

PubMed Abstract | CrossRef Full Text | Google Scholar

Glickman, N. S., and Yelon, D. (2002). Cardiac development in zebrafish: coordination of form and function. Semin. Cell. Dev. Biol. 13, 507–513. doi: 10.1016/s1084952102001040

PubMed Abstract | CrossRef Full Text | Google Scholar

Haack, T. B., Kopajtich, R., Freisinger, P., Wieland, T., Rorbach, J., Nicholls, T. J., et al. (2013). ELAC2 mutations cause a mitochondrial RNA processing defect associated with hypertrophic cardiomyopathy. Am. J. Hum. Genet. 93, 211–223. doi: 10.1016/j.ajhg.2013.06.006

PubMed Abstract | CrossRef Full Text | Google Scholar

Hance, N., Ekstrand, M. I., and Trifunovic, A. (2005). Mitochondrial DNA polymerase gamma is essential for mammalian embryogenesis. Hum. Mol. Genet. 14, 1775–1783. doi: 10.1093/hmg/ddi184

PubMed Abstract | CrossRef Full Text | Google Scholar

Howe, K., Clark, M. D., Torroja, C. F., Torrance, J., Berthelot, C., Muffato, M., et al. (2013). The zebrafish reference genome sequence and its relationship to the human genome. Nature 496, 498–503. doi: 10.1038/nature12111

PubMed Abstract | CrossRef Full Text | Google Scholar

Ihaka, R. G. R. (1996). R: A language for data analysis and graphics. J. Comput. Graph. Stat. 5, 299–314.

Google Scholar

Kimmel, C. B., Ballard, W. W., Kimmel, S. R., Ullmann, B., and Schilling, T. F. (1995). Stages of embryonic development of the zebrafish. Dev. Dyn. 203, 253–310. doi: 10.1002/aja.1002030302

PubMed Abstract | CrossRef Full Text | Google Scholar

Larbuisson, A., Dalcq, J., Martial, J. A., and Muller, M. (2013). Fgf receptors Fgfr1a and Fgfr2 control the function of pharyngeal endoderm in late cranial cartilage development. Differentiation 86, 192–206. doi: 10.1016/j.diff.2013.07.006

PubMed Abstract | CrossRef Full Text | Google Scholar

Larsson, N. G., Wang, J., Wilhelmsson, H., Oldfors, A., Rustin, P., Lewandoski, M., et al. (1998). Mitochondrial transcription factor A is necessary for mtDNA maintenance and embryogenesis in mice. Nat. Genet. 18, 231–236. doi: 10.1038/ng0398-231

PubMed Abstract | CrossRef Full Text | Google Scholar

Lindsey, J. (1999). Models for Repeated Measurements, 2nd Edn. Oxford: Oxford University Press.

Google Scholar

McGough, I. J., and Vincent, J. P. (2016). Exosomes in developmental signalling. Development 143, 2482–2493. doi: 10.1242/dev.126516

PubMed Abstract | CrossRef Full Text | Google Scholar

Metodiev, M. D., Thompson, K., Alston, C. L., Morris, A. A., He, L., Assouline, Z., et al. (2016). Recessive mutations in TRMT10C cause defects in mitochondrial RNA processing and multiple respiratory chain deficiencies. Am. J. Hum. Genet. 99:246. doi: 10.1016/j.ajhg.2016.06.013

PubMed Abstract | CrossRef Full Text | Google Scholar

Mi, H., Huang, X., Muruganujan, A., Tang, H., Mills, C., Kang, D., et al. (2017). PANTHER version 11: expanded annotation data from gene ontology and reactome pathways, and data analysis tool enhancements. Nucleic Acids Res. 45, D183–D189. doi: 10.1093/nar/gkw1138

PubMed Abstract | CrossRef Full Text | Google Scholar

Murayama, E., Kissa, K., Zapata, A., Mordelet, E., Briolat, V., Lin, H. F., et al. (2006). Tracing hematopoietic precursor migration to successive hematopoietic organs during zebrafish development. Immunity 25, 963–975. doi: 10.1016/j.immuni.2006.10.015

PubMed Abstract | CrossRef Full Text | Google Scholar

Otten, A. B., and Smeets, H. J. (2015). Evolutionary defined role of the mitochondrial DNA in fertility, disease and ageing. Hum. Reprod. Update 21, 671–689. doi: 10.1093/humupd/dmv024

PubMed Abstract | CrossRef Full Text | Google Scholar

Otten, A. B. C., Kamps, R., Lindsey, P., Gerards, M., Pendeville-Samain, M., Muller, M., et al. (2019). Tfam knockdown results in reduction of mtDNA copy number, OXPHOS deficiency and abnormalities in Zebrafish embryos. bioRxiv [preprint]. doi: 10.1101/843318

CrossRef Full Text | Google Scholar

Otten, A. B., Theunissen, T. E., Derhaag, J. G., Lambrichs, E. H., Boesten, I. B., Winandy, M., et al. (2016). Differences in strength and timing of the mtDNA bottleneck between zebrafish germline and non-germline cells. Cell Rep. 16, 622–630. doi: 10.1016/j.celrep.2016.06.023

PubMed Abstract | CrossRef Full Text | Google Scholar

Parisi, M. A., Xu, B., and Clayton, D. A. (1993). A human mitochondrial transcriptional activator can functionally replace a yeast mitochondrial HMG-box protein both in vivo and in vitro. Mol. Cell. Biol. 13, 1951–1961. doi: 10.1128/mcb.13.3.1951

PubMed Abstract | CrossRef Full Text | Google Scholar

Pauli, A., Montague, T. G., Lennox, K. A., Behlke, M. A., and Schier, A. F. (2015). Antisense oligonucleotide-mediated transcript knockdown in zebrafish. PLoS One 10:e0139504. doi: 10.1371/journal.pone.0139504

PubMed Abstract | CrossRef Full Text | Google Scholar

Powell, C. A., Nicholls, T. J., and Minczuk, M. (2015). Nuclear-encoded factors involved in post-transcriptional processing and modification of mitochondrial tRNAs in human disease. Front. Genet. 6:79. doi: 10.3389/fgene.2015.00079

PubMed Abstract | CrossRef Full Text | Google Scholar

Richardson, R., Tracey-White, D., Webster, A., and Moosajee, M. (2017). The zebrafish eye-a paradigm for investigating human ocular genetics. Eye 31, 68–86. doi: 10.1038/eye.2016.198

PubMed Abstract | CrossRef Full Text | Google Scholar

Santos, T. A., El Shourbagy, S., and St John, J. C. (2006). Mitochondrial content reflects oocyte variability and fertilization outcome. Fertil. Steril. 85, 584–591. doi: 10.1016/j.fertnstert.2005.09.017

PubMed Abstract | CrossRef Full Text | Google Scholar

Semino, C. E., and Allende, M. L. (2000). Chitin oligosaccharides as candidate patterning agents in zebrafish embryogenesis. Int. J. Dev. Biol. 44, 183–193.

Google Scholar

Shutt, T. E., Bestwick, M., and Shadel, G. S. (2011). The core human mitochondrial transcription initiation complex: it only takes two to tango. Transcription 2, 55–59. doi: 10.4161/trns.2.2.14296

PubMed Abstract | CrossRef Full Text | Google Scholar

Stackley, K. D., Beeson, C. C., Rahn, J. J., and Chan, S. S. (2011). Bioenergetic profiling of zebrafish embryonic development. PLoS One 6:e25652. doi: 10.1371/journal.pone.0025652

PubMed Abstract | CrossRef Full Text | Google Scholar

Thomas, P. D., Campbell, M. J., Kejariwal, A., Mi, H., Karlak, B., Daverman, R., et al. (2003). PANTHER: a library of protein families and subfamilies indexed by function. Genome Res. 13, 2129–2141. doi: 10.1101/gr.772403

PubMed Abstract | CrossRef Full Text | Google Scholar

Torrent, M., Chalancon, G., de Groot, N. S., Wuster, A., and Madan Babu, M. (2018). Cells alter their tRNA abundance to selectively regulate protein synthesis during stress conditions. Sci. Signal. 11:eaat6409. doi: 10.1126/scisignal.aat6409

PubMed Abstract | CrossRef Full Text | Google Scholar

Ventura-Clapier, R., Garnier, A., Veksler, V., and Joubert, F. (2011). Bioenergetics of the failing heart. Biochim. Biophys. Acta. 1813, 1360–1372. doi: 10.1016/j.bbamcr.2010.09.006

PubMed Abstract | CrossRef Full Text | Google Scholar

Wagener, F. A., Volk, H. D., Willis, D., Abraham, N. G., Soares, M. P., Adema, G. J., et al. (2003). Different faces of the heme-heme oxygenase system in inflammation. Pharmacol. Rev. 55, 551–571. doi: 10.1124/pr.55.3.5

PubMed Abstract | CrossRef Full Text | Google Scholar

Wai, T., Ao, A., Zhang, X., Cyr, D., Dufort, D., and Shoubridge, E. A. (2010). The role of mitochondrial DNA copy number in mammalian fertility. Biol. Reprod. 83, 52–62. doi: 10.1095/biolreprod.109.080887

PubMed Abstract | CrossRef Full Text | Google Scholar

Wan, J., Yourshaw, M., Mamsa, H., Rudnik-Schoneborn, S., Menezes, M. P., Hong, J. E., et al. (2012). Mutations in the RNA exosome component gene EXOSC3 cause pontocerebellar hypoplasia and spinal motor neuron degeneration. Nat. Genet. 44, 704–708. doi: 10.1038/ng.2254

PubMed Abstract | CrossRef Full Text | Google Scholar

Yamamoto, T., Iwata, H., Goto, H., Shiratuki, S., Tanaka, H., Monji, Y., et al. (2010). Effect of maternal age on the developmental competence and progression of nuclear maturation in bovine oocytes. Mol. Reprod. Dev. 77, 595–604. doi: 10.1002/mrd.21188

PubMed Abstract | CrossRef Full Text | Google Scholar

Zhang, J., and Hamza, I. (2018). Zebrafish as a model system to delineate the role of heme and iron metabolism during erythropoiesis. Mol. Genet. Metab. 128, 204–212. doi: 10.1016/j.ymgme.2018.12.007

PubMed Abstract | CrossRef Full Text | Google Scholar

Zhang, X. Y., and Rodaway, A. R. (2007). SCL-GFP transgenic zebrafish: in vivo imaging of blood and endothelial development and identification of the initial site of definitive hematopoiesis. Dev. Biol. 307, 179–194. doi: 10.1016/j.ydbio.2007.04.002

PubMed Abstract | CrossRef Full Text | Google Scholar