Zebrafish Models of Autosomal Recessive Ataxias

cells Review Zebrafish Models of Autosomal Recessive Ataxias Ana Quelle-Regaldie 1, Daniel Sobrido-Cameán2,† , Antón Barreiro-Iglesias 2,‡ , María Jesús Sobrido 3,‡ and Laura Sánchez 1,4,*,‡   Citation: Quelle-Regaldie, A.; Sobrido-Cameán, D.; Barreiro-Iglesias, A.; Sobrido, M.J.; Sánchez, L. Zebrafish Models of Autosomal Recessive Ataxias. Cells 2021,10, 836. https://doi.org/ 10.3390/cells10040836 Academic Editor: Sylvie Schneider-Maunoury Received: 9 March 2021 Accepted: 6 April 2021 Published: 8 April 2021 Publisher’s Note: MDPI stays neutral with regard to jurisdictional claims in published maps and institutional affiliations. Copyright: © 2021 by the authors. Licensee MDPI, Basel, Switzerland. This article is an open access article distributed under the terms and conditions of the Creative Commons Attribution (CC BY) license (https:// creativecommons.org/licenses/by/ 4.0/). 1Department of Zoology, Genetics and Physical Anthropology, Faculty of Veterinary Science, Universidade de Santiago de Compostela, 27002 Lugo, Spain; [email protected] 2Department of Functional Biology, CIBUS, Faculty of Biology, Universidade de Santiago de Compostela, 15782 Santiago de Compostela, Spain; [email protected] (D.S.-C.); anton.barreir[email protected] (A.B.-I.) 3Instituto de Investigación Biomédica de A Coruña (INIBIC), Servicio Galego de Saúde, 15006 A Coruña, Spain; [email protected] 4Preclinical Animal Models Group, Health Research Institute of Santiago de Compostela (IDIS), 15706 Santiago de Compostela, Spain *Correspondence: [email protected] † Current address: Department of Zoology, University of Cambridge, Cambridge CB2 3EJ, UK. ‡ These authors contributed equally to the manuscript. Abstract: Autosomal recessive ataxias are much less well studied than autosomal dominant ataxias and there are no clearly defined systems to classify them. Autosomal recessive ataxias, which are characterized by neuronal and multisystemic features, have significant overlapping symptoms with other complex multisystemic recessive disorders. The generation of animal models of neurodegenerative disorders increases our knowledge of their cellular and molecular mechanisms and helps in the search for new therapies. Among animal models, the zebrafish, which shares 70% of its genome with humans, offer the advantages of being small in size and demonstrating rapid development, making them optimal for high throughput drug and genetic screening. Furthermore, embryo and larval transparency allows to visualize cellular processes and central nervous system development in vivo . In this review, we discuss the contributions of zebrafish models to the study of autosomal recessive ataxias characteristic phenotypes, behavior, and gene function, in addition to commenting on possible treatments found in these models. Most of the zebrafish models generated to date recapitulate the main features of recessive ataxias. Keywords: zebrafish; hereditary recessive ataxias; neurodegenerative disorders; genetic edition 1. Introduction Hereditary ataxias are a heterogeneous group of rare neurodegenerative disorders caused by progressive degeneration of the cerebellum and spinocerebellar tracts resulting in loss of balance and coordination. Classification of hereditary ataxias has been problematic due to phenotype overlap and the broad number of syndromes that manifest ataxia as a common symptom, such as hereditary spastic paraplegias and polyneuropathies. However, the development of novel molecular techniques has made it possible to classify ataxias based on genetics [ 1 ]. Ataxias can be divided into autosomal dominant, autosomal recessive and X-linked ataxias [2,3]. Unlike autosomal dominant ataxias [ 4 ], autosomal recessive ataxias have been less well studied. Autosomal recessive ataxias are more difficult to classify because, contrary to autosomal dominant ataxias, they are not organized with a numerical naming system. The term spinocerebellar ataxia autosomal recessive (SCAR) was recently used to designate novel ataxias, but it is based only on locus discovery and it does not include the previously identified and more frequent recessive ataxias. In addition, many recessive multisystemic or complex metabolic disorders present ataxia as a symptom [ 2 , 3 ]. There are more than 100 loci related with recessive ataxias. The development of next generation sequencing Cells 2021,10, 836. https://doi.org/10.3390/cells10040836 https://www.mdpi.com/journal/cells Cells 2021,10, 836 2 of 28 technology helped to classify and discover new recessive ataxias [ 5 ]. Autosomal recessive ataxias are a group of complex neuronal disorders usually showing early onset, involving central and peripheral nervous systems. They often affect other systems and organs and cause—among others—symptoms such as: peripheral sensorimotor neuropathy; pyramidal and extrapyramidal involvement; oculomotor defects; retinopathy; cognitive impairment; metabolism abnormalities; seizures and hypogonadism [ 2 , 6 ]. The pathogenesis of autosomal recessive ataxias is associated with loss of function of the related proteins, which are involved in a broad number of pathways such as: mitochondrial metabolism and function; metabolic homeostasis; DNA repair; the cell cycle; RNA processing; protein folding; synaptic morphology and the synaptogenesis of Purkinje cells [3,7,8]. The use of animal models of neurodegenerative disorders can, at least partially, recapitulate the human disease to help unravel the molecular and cellular mechanisms responsible and represent a first step in developing therapies for diseases that do not yet have available treatments [ 9 ]. For example, in ataxias, Purkinje cell degeneration and motor deficits were demonstrated in several mice models [10]. The zebrafish (Danio rerio) shares 70% of its genome with humans [ 11 ] and is an emerging animal model that is gaining popularity in the study of a wide range of medical conditions, such as cancer [ 12 ], neurogenetic diseases [ 13 ], psychiatry disorders [ 14 ], cardiovascular illnesses [ 15 ] and traumatic injuries [ 16 , 17 ]. Its many advantages include: easy genetic manipulation; the capacity to perform high throughput drug and genetic screening; optical transparency that allows for visualizing the central nervous system (CNS) and cellular processes. In addition, behavioral patterns are measurable and easy to evaluate, including high order behaviors such as memory, conditioned responses and social behaviors [ 18 ]. The organization of the CNS of the zebrafish is similar to mammals, including humans. Moreover, most genes related to neural activity or development show similar functions in mammals and zebrafish. On the other hand, the zebrafish model has the advantage of having a reduced CNS complexity, which simplifies functional studies [19]. The development of zebrafish loss of function models is easily achieved by transient knock-down with antisense morpholinos that block translation or splicing [ 20 ]. Permanent knock-out models are created with mutagens such as N-ethyl-N-nitrosourea (ENU) [ 21 ], transgenesis or genetic edition via the use of TALENs (Transcription activator-like effector nucleases), zinc finger nucleases or the recently discovered CRISPR/Cas9 techniques [22] (Figure 1). In this review, we used the Bird classification [ 23 ] of ataxias (which includes recently discovered ataxias) to search zfin (https://zfin.org/ (accessed on 27 January 2021)) and PubMed (https://pubmed.ncbi.nlm.nih.gov/ (accessed on 27 January 2021)) databases for zebrafish models targeting genes that cause recessive disorders with cerebellar ataxia among their clinical manifestations. These data are compiled in Supplemental Table S1. We discuss the zebrafish models created for the more common recessive ataxias, recessive ataxias that are relatively more uncommon (only present in a few families), and recessive disorders that cause abnormalities of cerebellar development and prominent ataxia. The molecular basis and relevant clinical data of the diseases discussed in the present review are summarized in Table 1(more frequent autosomal recessive ataxias in green, less frequent autosomal recessive ataxias in blue and recessive inherited disorders related to ataxia in orange). Cells 2021,10, 836 3 of 28 Cells 2021, 10, x FOR PEER REVIEW 3 of 29 Figure 1. Main techniques for generating zebrafish loss of function models. Table 1. Summary of molecular mechanisms and main clinical features of the ataxias discussed in this article. Disease Gene Protein Function Clinical Features Other Than Ataxia * References Ataxia-telangiect asia (AT) ATM Cellular responses to DNA damage and cell cycle control Oculocutaneous telangiectasia, radiosensitivity, predisposition to lymphoid malignancies, cellular and humoral immunodeficiency [24] Boucher–Neuhä user syndrome; Spastic paraplegia type 39 (SPG39) PNPLA6 Phospholipase Hypogonadotropic hypogonadism, chorioretinal dystrophy [25] Marinesco-Sjögr en syndrome SIL1 Nuclear exchange factor for the endoplasmic reticulum resident chaperone BiP Cataracts, skeletal muscle myopathy, developmental delay [26] Spinocerebellar ataxia autosomal recessive type 20 (SCAR20) SNX14 Autophagosome function Intellectual disability, coarse facial features, hearing loss, epilepsy, macrocephaly [27] Ataxia with isolated vitamin E deficiency (AVED) TTPA Distribution of vitamin E Hyporeflexia, decreased vibration sense, cardiomyopath, retinitis pigmentosa [28] Wolfram WFS1 Membrane Mental retardation, seizures, [29,30] Figure 1. Main techniques for generating zebrafish loss of function models. Table 1. Summary of molecular mechanisms and main clinical features of the ataxias discussed in this article. Disease Gene Protein Function Clinical Features Other Than Ataxia * References Ataxia-telangiectasia (AT) ATM Cellular responses to DNA damage and cell cycle control Oculocutaneous telangiectasia, radiosensitivity, predisposition to lymphoid malignancies, cellular and humoral immunodeficiency [24] Boucher–Neuhäuser syndrome; Spastic paraplegia type 39 (SPG39) PNPLA6 Phospholipase Hypogonadotropic hypogonadism, chorioretinal dystrophy [25] Marinesco-Sjögren syndrome SIL1 Nuclear exchange factor for the endoplasmic reticulum resident chaperone BiP Cataracts, skeletal muscle myopathy, developmental delay [26] Spinocerebellar ataxia autosomal recessive type 20 (SCAR20) SNX14 Autophagosome function Intellectual disability, coarse facial features, hearing loss, epilepsy, macrocephaly [27] Ataxia with isolated vitamin E deficiency (AVED) TTPA Distribution of vitamin E Hyporeflexia, decreased vibration sense, cardiomyopath, retinitis pigmentosa [28] Wolfram syndrome (WFS) WFS1 Membrane trafficking, endoplasmic reticulum stress and calcium homeostasis Mental retardation, seizures, psychiatric symptoms, pigmentary retinopathy, Diabetes mellitus, optic atrophy, sensorineural hearing loss, urinary tract abnormalities [29,30] Polyneuropathy, hearing loss, ataxia, retinitis pigmentosa and cataract (PHARC) ABHD12 Endocannabinoid and phospholipid metabolism Cataracts, hearing loss, retinitis pigmentosa, demyelinating sensorimotor polyneuropathy [31] Cayman ataxia ATCAY Neural development Hypotonia, psychomotor retardation [32] Spinocerebellar ataxia autosomal recessive type 25 (SCAR25) ATG5 Autophagy Mental retardation, developmental delay [33] Cells 2021,10, 836 4 of 28 Table 1. Cont. Disease Gene Protein Function Clinical Features Other Than Ataxia * References Spastic paraplegia type 76 (SPG76) CAPN1 Neuronal plasticity, migration, microtubular regulation Skeletal abnormalities, peripheral neuropathy, amyotrophy, spastic paraplegia [34] Spinocerebellar ataxia autosomal recessive (SCAR17) CWF19L1 Cell Cycle Control Developmental delay, mental retardation [35] EAST syndrome KCNJ10 Potassium channel Short stature, epilepsy, sensorineural deafness, mental retardation, renal tubulopathy [36,37] Poretti-Boltshauser syndrome LAMA1 Cell attachment, migration Retinal dystrophy [38] Mitochondrial recessive ataxia syndrome (MIRAS) POLG Catalytic subunit of mitochondrial DNA polymerase Ophthalmoplegia, polyneuropathy, myopathy, encephalopathy, liver failure, muscle pain, sensorineural hearing loss, epilepsy [39,40] Pancreatic and cerebellar agenesis (PACA) PTF1A Pancreatic development Neonatal diabetes mellitus, pancreatic and cerebellar agenesis [41] Gordon Holmes syndrome RNF216 Ubiquitination Chorea, dementia, hypogonadotropic hypogonadism [42] Childhood-onset neurodegeneration with ataxia, dystonia, and gaze palsy (NADGP) SQSTM1 Intracellular signalling, oxidative stress response, apoptosis and autophagy Dystonia, gaze palsy, dyskinesia, cognitive decline [43] Spinocerebellar ataxia autosomal recessive type 7 (SCAR7), Ceroid lipofuscinosis neuronal 2 (CLN2) TPP1 Serine peptidase SCAR7: Slowly progressive spasticity CLN2: Rapidly progressive myoclonus, developmental regression, early death, epilepsy, loss of vision [44] Spinocerebellar ataxia autosomal recessive type 24 (SCAR24) UBA5 Ubiquitin-like Cataracts, demyelinating sensorimotor neuropathy [45] Galloway-Mowat syndrome WDR73 Unknown Intellectual disability, short stature, microcephaly, facial dysmorphism, hypotonia, nephrotic synrome, cataracts, skin hypopigmentation [46] Spinocerebellar ataxia autosomal recessive type 12 (SCAR12) WWOX DNA repair Epilepsy, mental retardation, developmental delay. microcephaly [47–49] Niemann–Pick disease type C (NPC) NPC1 Cholesterol trafficking Learning difficulties, neuropsychiatric symptoms, dementia, seizures, dystonia, supranuclear gaze palsy, neonatal cholestasis, hepatosplenomegaly [50] Cerebellar ataxia and mental retardation with or without quadrupedal locomotion 3 (CAMRQ3) CA8 Unknown Mental retardation quadrupedal gait [51,52] Joubert syndrome Several genes Diverse functions Hypotonia, Developmental delay, oculomotor apraxia, breathing dysregulation, retinal abnormalities, renal cysts, polydactily, hepatic fibrosis [53] Pontocerebellar hypoplasia Several genes Diverse functions Hypoplasia of the cerebellum or the ventral pons, progressive microcephaly, motorneuron disease, resiratory insuficiency, mental retardation [54] * Cerebellar ataxia is a feature of all the disorders in this table. Not all listed clinical manifestations are necessarily present in every patient with the disorder. EAST syndrome: epilepsy, ataxia, sensorineural deafness and tubulopathy. Cells 2021,10, 836 5 of 28 2. Materials and Methods Articles were found in the zfin database (https://zfin.org/ (accessed on 27 January 2021 )) by searching for zebrafish models of genes that cause recessive ataxias as described in the classification of Bird [23] and some recessive disorders that have prominent ataxia. The PubMed database (https://pubmed.ncbi.nlm.nih.gov/ (accessed on 27 January 2021 )) was used to find additional models related to these diseases by searching for “zebrafish” and “name of the disease”. The articles included in this review were published before 27 January 2021. 3. Results The genes responsible for the diseases discussed here are implicated in a broad number of signaling pathways and cellular processes that are summarized in Figure 2. In the following sections, we will review the main findings obtained with zebrafish models for each of these genes. Cells 2021, 10, x FOR PEER REVIEW 6 of 29 The first ataxia-telangiectasia zebrafish model was generated with morpholinos and reproduced the role of ATM in the DNA damage response [55]. Atm morphants exhibit normal development but when a radiation dose of 8 Gy was applied to 6 hpf atm morphants, abnormal development with retardation was observed. Atm irradiated morphants exhibited no pigmentation, a lack of yolk extension, and extreme ventral body curvature and died by 72 hpf. Higher amounts of atm morpholino, combined with radiation, increased mortality of embryos by 48 hpf and induced more severe curvature and absence of yolk extension phenotypes. This phenotype caused by irradiation was not seen in embryos injected with a control morpholino, which means that deficiency in atm leads to increased radiosensitivity [55]. Figure 2. Main functions of genes related to recessive ataxias. Recently, an atm zebrafish mutant was developed which did not show neurodegenerative defects but developed exclusively as infertile males [56]. Infertility is a characteristic of some AT patients. Disabling the apoptosis pathway with a p53 mutation rescued the all-male phenotype, but not infertility. In addition, atm-p53 double mutants showed quick tumor formation, which suggests that atm acts as a tumor suppressor and is involved in maintaining genomic stability. Surprisingly, atm mutant embryos did not display the radiosensitivity observed in atm morphant embryos. This is probably due to compensation mechanisms [56]. These results indicate that zebrafish models of atm can be used to analyze the function of ATM in the DNA damage response but not for neurodegeneration. • Boucher–Neuhäuser syndrome and spastic paraplegia type 39 (SPG39). Mutations in the PNPLA6 (patatin like phospholipase domain containing 6) gene cause SPG39 and Boucher–Neuhäuser syndrome which express similar symptoms [25]. Other syndromes that have been related with mutations in PNPLA6 include: (i) Oliver–McFarlane syndrome, the features of which consist of trichomegaly, congenital hypopituitarism and retinal degeneration with choroidal atrophy; (ii) Laurence–Moon syndrome, which presents in a similar manner, though with progressive spinocerebellar ataxia and spastic paraplegia, and without trichomegaly [57]. Pnpla6 zebrafish morphants have been shown to exhibit a curly tail that is dose-dependent. The head–tail distance was shorter in morphants and they also had abnormal eye development and reduced otic vesicle size. Morphant eyes were smaller than in controls and some of them had unclosed eye fissures [57,58]. In addition, some pnpla6 morphants showed midbrain–hindbrain boundary defects, swelling of the pericardium, reduced heart rate and reduced blood flow [58]. Normal PNPLA6 human Figure 2. Main functions of genes related to recessive ataxias. 3.1. Autosomal Recessive Cerebellar Ataxias •Ataxia-telangiectasia (AT). AT is an infantile onset multisystemic disease produced by mutations in the ATM gene (ataxia-telangiectasia mutated), which is involved in cellular responses to DNA damage and cell cycle control [24]. The first ataxia-telangiectasia zebrafish model was generated with morpholinos and reproduced the role of ATM in the DNA damage response [ 55 ]. Atm morphants exhibit normal development but when a radiation dose of 8 Gy was applied to 6 hpf atm morphants, abnormal development with retardation was observed. Atm irradiated morphants exhibited no pigmentation, a lack of yolk extension, and extreme ventral body curvature and died by 72 hpf. Higher amounts of atm morpholino, combined with radiation, increased mortality of embryos by 48 hpf and induced more severe curvature and absence of yolk extension phenotypes. This phenotype caused by irradiation was not seen in embryos injected with a control morpholino, which means that deficiency in atm leads to increased radiosensitivity [55]. Recently, an atm zebrafish mutant was developed which did not show neurodegenerative defects but developed exclusively as infertile males [ 56 ]. Infertility is a characteristic of some AT patients. Disabling the apoptosis pathway with a p53 mutation rescued the all-male phenotype, but not infertility. In addition, atm-p53 double mutants showed quick tumor formation, which suggests that atm acts as a tumor suppressor and is involved Cells 2021,10, 836 6 of 28 in maintaining genomic stability. Surprisingly, atm mutant embryos did not display the radiosensitivity observed in atm morphant embryos. This is probably due to compensation mechanisms [ 56 ]. These results indicate that zebrafish models of atm can be used to analyze the function of ATM in the DNA damage response but not for neurodegeneration. •Boucher–Neuhäuser syndrome and spastic paraplegia type 39 (SPG39). Mutations in the PNPLA6 (patatin like phospholipase domain containing 6) gene cause SPG39 and Boucher–Neuhäuser syndrome which express similar symptoms [ 25 ]. Other syndromes that have been related with mutations in PNPLA6 include: (i) Oliver–McFarlane syndrome, the features of which consist of trichomegaly, congenital hypopituitarism and retinal degeneration with choroidal atrophy; (ii) Laurence–Moon syndrome, which presents in a similar manner, though with progressive spinocerebellar ataxia and spastic paraplegia, and without trichomegaly [57]. Pnpla6 zebrafish morphants have been shown to exhibit a curly tail that is dosedependent. The head–tail distance was shorter in morphants and they also had abnormal eye development and reduced otic vesicle size. Morphant eyes were smaller than in controls and some of them had unclosed eye fissures [ 57 , 58 ]. In addition, some pnpla6 morphants showed midbrain–hindbrain boundary defects, swelling of the pericardium, reduced heart rate and reduced blood flow [ 58 ]. Normal PNPLA6 human mRNA was able to rescue the phenotype but not PNPLA6 human mRNA without the catalytic domain. This means that the phenotype in pnpla6 morphants was due to reduced esterase activity [ 58 ]. Likewise, co-injection with human mRNA with known mutations of SPG39, Oliver–McFarlane syndrome or Laurence–Moon syndrome, did not rescue the phenotype [ 57 ]. Motor neurons and spinal motor neuron numbers were reduced in pnpla6 morphant zebrafish. Aberrant motor axon branching was also observed, which seemed to be truncated and failed to join the ventral muscles. An increase in apoptosis was observed in this model, especially in the CNS, that was not rescued with co-injection of p53 morpholino. Cell cultures of pnpla6 morphant spinal neurons were performed to confirm that the cause of impaired motor neuron development was not the presence of a deformed body. Chimeric embryos transplanted with one cell stage pnpla6 morphant cells also developed axon defects. Mauthner neurons, interneurons and sensory neurons showed no morphological differences in pnpla6 morphants. BMP (bone morphogenetic protein) signaling was studied by blocking the kinase activity of BMP receptors with dorsomorphin, which resulted in phenotype rescue in pnpla6 morphants. This indicates that BMP was overexpressed in pnpla6 knock-down and that this caused at least part of the morphant phenotype [ 58 ]. Although these results revealed the neurological consequences of pnpla6 dysfunction and a relation with BMP overexpression, it is necessary to develop a mutant zebrafish model to see if this will reproduce the phenotype observed with morpholinos. •Marinesco–Sjögren syndrome. Marinesco–Sjögren syndrome is a multisystemic early onset disorder caused by mutations in the SIL1 (SIL1 Nucleotide Exchange Factor) gene, which encodes a nuclear exchange factor for the endoplasmic reticulum resident chaperone BiP (binding immunoglobulin protein) [26]. Zebrafish morphants for sil1 showed abnormal shape and small eyes. Birefringence assays revealed abnormal skeletal muscle structure at 4 dpf in morphant embryos. The phenotype was rescued by the co-injection of sil1 wild type mRNA. Histological examination revealed deformed beta-dystroglycan expression at myosepta with a less clear V-shaped structure and disturbed formation in sil1 morphants. Reduced numbers of Purkinje cells were observed in sil1 morphant embryos in comparison with controls. Interestingly, sil1 morphants displayed an increase in levels of BiP, the lipidated form of Lc3 (light chain 3) and caspase 3, which are markers associated with endoplasmic reticulum stress, autophagy and apoptosis, respectively [59]. Sil1 deficiency in peripheral nerves and neuromuscular junctions was also studied using sil1 morpholino knock-down in zebrafish. Sil1 morphants demonstrated disrupted Cells 2021,10, 836 7 of 28 synapse formation along the vertical myosepta, with remarkable disorganization of presynaptic branching across the muscle fibers of the myotomes. Analysis of myelinating Schwann cells did not show significant differences between sil1 morphants and control zebrafish [60]. These morphant models revealed neural damage, abnormalities in the skeletal muscle and neuromuscular junctions, and activation of endoplasmic reticulum stress, autophagy and apoptosis, which are features of Marinesco–Sjögren patients. The development of a mutant zebrafish model will assist in the search for treatments and confirm the morphant phenotypes. •Spinocerebellar ataxia autosomal recessive type 20 (SCAR20). SCAR20 is caused by mutations in the sorting nexin 14 gene (SNX14), which is required for autophagosome clearance [27]. Snx14 zebrafish morphants displayed loss of neural tissue volume and reduced number of Purkinje cells that was rescued with co-injection with human SNX14 mRNA. In addition, morpholino injection in a reporter line that expressed GFP in the hindbrain revealed a significant reduction in hindbrain size in morphant embryos. An increase in apoptosis across the neural tissue was also seen. Transmission electron microscopy analysis of snx14 morphant neural cells also revealed an accumulation of autophagic structures. These data suggest that snx14 mutations caused neuronal cell death associated with impaired autophagic degradation and apoptosis [27]. Surprisingly, a more recent study using snx14 morpholinos in zebrafish did not detect morphological defects or motor neuron abnormalities. In the same study, an snx14 zebrafish knock-out model was examined, and no morphological or neuronal abnormalities were detected, not even when maternal zygotic mutants were analyzed. Behavioral analysis also showed that mutant snx14 zebrafish did not develop a locomotor phenotype. As SNX14 mutations had been reported to disrupt neutral lipid metabolism, lipids from 4 dpf zebrafish were extracted and analyzed through total fatty acids lipidomic profiling. It was observed that total fatty acids from neutral lipids (both saturated and unsaturated) were elevated in snx14 knock-out embryos in comparison with wild type and heterozygous embryos. These results confirm that SNX14 has a conserved role in lipid biogenesis [61]. The discrepancies in these studies could be because Bryant et al. [ 61 ] used sub toxic doses of morpholinos. Morpholinos are only considered reliable when a mutant model supports morpholino findings due to the previously observed off target effects of morpholinos [ 62 ]. In addition, the premature stop codon of mutants resulted in a nonsense mediated decay that upregulated homologous gene sequences that rescue the phenotype. The consequence of the mutation at the protein level could not be demonstrated in zebrafish because there was no SNX14 antibody available that could react with the corresponding zebrafish protein [61]. •Ataxia with isolated vitamin E deficiency (AVED). AVED is caused by mutations in the α tocopherol transfer protein (TTPA) gene which is responsible for the distribution of vitamin E [28]. Ttpa is expressed in the zebrafish brain, eye and tailbud. Experiments with morpholinos in zebrafish showed significant developmental defects at 1 dpf along the anterior/posterior axis, with truncated tail and brain and eye malformations. However, time lapse analysis reported normal development during blastula formation, epiboly and gastrulation until 12 hpf, when the tppa morphant eye began to display tissue darkening, indicating the initiation of improper head growth. Co-injection with a p53 morpholino did not affect the phenotype [63]. Previous studies with a vitamin E-deficient diet in adult zebrafish caused a decreased startle response that suggested the occurrence of neurological defects. Embryos produced by zebrafish E depleted adults displayed increased mortality and morphological abnormalities such as cranial malformations, a bent anterior–posterior axis, pericardial edema, swim bladder malformations and yolk-sac edema [ 64 , 65 ]. Surviving vitamin E deficient Cells 2021,10, 836 8 of 28 embryos of 24 hpf had somite malformations and stunted fin formation. At 48 hpf embryos developed acute pericardial and yolk sac edema. Collagen sheath notochord markers col2a1a (collagen, type II, alpha 1a) and col9a2 (collagen, type IX, alpha 2) showed bent axes. Surprisingly, it was demonstrated that a vitamin E deficient diet did not affect the localization or expression of ttpa but affected brain structure. In addition, tppa was found to be expressed at 24 hpf in the midbrain–hindbrain boundary and pax2a (paired box 2a) (which defines the midbrain–hindbrain boundary) expressed a diffused signal at 12 and 24 hpf [65]. Future studies with mutants may support the discoveries made with morpholinos and with a vitamin E deficient diet. •Wolfram syndrome (WFS). WFS is a juvenile progressive neurodegenerative disorder caused by mutations in WFS1, which encodes the wolframin protein. This is an endoplasmic reticulum membraneembedded protein related to membrane trafficking, endoplasmic reticulum stress and calcium homeostasis [29,30]. Zebrafish have two paralogous genes of WFS1,wfs1a and wfs1b. The first knockdown of wfs1b was created during an assessment of genes that are relevant to diabetes type 2. Wfs1b knock-down caused a reduction in pancreatic β -islet cells and reduced insulin expression, suggesting that WFS1 is involved in glucose homeostasis [66]. A broader study of zebrafish models was performed by Cairns [ 67 ]. Morpholinos for wfs1a and wfs1b caused abnormal eye, brain and otoliths, although the wfs1b phenotype was more pathological. Co-injection of the two wfs1 morpholinos caused lethality in most embryos and p53 morpholino co-injection did not rescue the phenotype. CRISPR/Cas9 models of wfs1a and wfs1b genes displayed delayed development and smaller otoliths. Wfs1 knock-outs, particularly the wfs1b knock-out, showed significant delay in neuronal growth. At 24 hpf, wfs1b displayed shortened motor axons that seemed to be corrected at 48 hpf. Expression of acetylcholine receptors developed normally in both wfs1 knock-outs, indicating that muscular growth was normal. Acetylcholinesterase activity was reduced in wfs1a and wfs1b knock-out embryos, which suggested reduced brain activity, but only was reduced in the wfs1b knock-out at 12 months, suggesting defective neurogenesis in wfs1b knock-out fish. Moreover, mutants had a smaller cerebellum than the wild types. Spontaneous movements of wfs1b knock-out zebrafish were significantly higher at 24 hpf and significantly lower at 48 hpf, as compared to both controls and wfs1a knock-outs. As no differences were detected in the muscle fiber structure, this was associated with problems related to neuronal signaling in response to tactile stimulation. Mitochondrial trafficking was affected in both wfs1 knock-outs and mitochondrial respiration was reduced in the wfs1b knock-out. Mitochondrial complex I protein expression was reduced in wfs1a and wfs1b knock-out whole embryos and muscle and also in the brain in wfs1b knock-out embryos. However, Ca 2+ uptake and mitochondrial DNA levels remained normal in both wfs1 knock-outs. Heat shock—to induce endoplasmic reticulum stress— increased the death rate in the two wfs1 knock-outs, suggesting increased apoptosis due to increased endoplasmic reticulum stress response. BiP protein expression was shown to be upregulated in both heat shocked and untreated wfs1 knock-outs. Wfs1b knock-out adult zebrafish displayed less locomotion when they were isolated in order to record their behavior, which suggested increased anxiety. Wfs1b knock-out adults had a significantly lower blood glucose level and lower fertility than wfs1a and wild type fish. In addition, both knock-outs had a significantly lower number of retinal ganglion cells than wild type fish at 4 months and this number decreased even more at 12 months. Wfs1b retinal ganglion cell numbers were also significantly lower than in wfs1a. Less eye movement and a thinner optic nerve were also observed in the wfs1b knock-outs at 12 months. The fact that wfs1b displayed the most severe phenotype, replicating some of the symptoms of wolfram syndrome patients, could be due to its expression in eyes and neural tissue, unlike wfs1a which was only found to be expressed in muscle tissue [ 67 ]. The use of these models reproducing the pathological mechanisms of patients with WFS may help to find a therapy to Wolfram syndrome. Cells 2021,10, 836 9 of 28 3.2. Less Frequent Autosomal Recessive Ataxias •Polyneuropathy, hearing loss, ataxia, retinitis pigmentosa and cataract (PHARC). PHARC is produced by mutations in ABHD12, which encodes the abhydrolase domain containing protein 12, an enzyme related to endocannabinoid and phospholipid metabolism and that has essential functions in the central and peripheral nervous systems [31]. A morpholino for the ABHD12 gene was generated as part of a study on neuropathy candidate genes related to Charcot–Marie–Tooth disease. Abhd12 morphant embryos had aberrant motor neuron axon extension, pathfinding and branching, with an abnormal morphology of peripheral neurons [68]. In a more recent study, Abhd12 zebrafish morphants injected with a splice block morpholino displayed two phenotypes: mild and moderate. The moderate phenotype included severe microphthalmia, microcephaly and reduced body length due to a significant reduction in head size. From 3 dpf, both morphant phenotypes did not have spontaneous free-swimming activity. The moderate phenotype did not display any locomotor activity in a touch-evoked escape response and mild phenotype animals exhibited impaired locomotor activity similar to ataxia. None of these phenotypes were rescued after p53 morpholino co-injection. Axonogenesis and motor neuron axon outgrowth was normal in abhd12 morphants at 3 dpf. However, myelination of the axonal tracks was severely impaired in abhd12 morphants at 5 dpf. Neuromasts suffer a large reduction in the anterior and posterior lateral line and auditory system in comparison with controls. Normal Purkinje cell differentiation was observed, while the morphology of the Purkinje cell layer was affected. A strong impairment of retinal architecture and stratification, absence of lens clarification and a high decrease in retinotectal projections was also found in abhd12 morphants. Injection of a translation block morpholino caused a severe phenotype with exacerbation of morphological symptoms, a curved tail and the absence of spontaneous swimming. Co-injection with abhd12 mRNA of wild type zebrafish embryos or human ABHD12 mRNA rescued the phenotype of morphant embryos. However, co-injection with human ABHD12 mRNA encoding one missense or nonsense mutation associated with PHARC could not restore the normal phenotype [ 69 ]. The molecular consequences of blocking translation seemed to be worse than when blocking mRNA splicing. This may be due to the different biological role of some parts of the truncated protein. These models reproduced several of the symptoms of PHARC patients, such as ataxia, disruption of retinal architecture and a reduction in mechanosensory hair cells in the inner ear and lateral line. However, it is necessary to generate mutant models to confirm that these findings were not caused by off-target effects and to search for therapies. •Cayman ataxia. Cayman ataxia is a recessive congenital ataxia restricted to the Grand Cayman Island. Cayman ataxia is caused by mutations in the ATCAY gene, which encodes a neuronal protein called Caytaxin [32]. Atcay morphants displayed reduced motor axon length in a dose-dependent manner at 72 hpf. This phenotype was rescued with mouse atcay mRNA and also by mouse VAchT (vesicular acetylcholine transporter) mRNA, which acts downstream of acetylcholine synthesis and release. This indicates that atcay regulates neurite outgrowth through cholinergic signaling. Interestingly, knock-down of chat (choline acetyltransferase, which produces acetylcholine) or acl (ATP citrate lyase, an enzyme that produces acetyl-CoA for lipogenesis, cholesterol genesis and acetylcholine synthesis in the citosol) genes also caused shorter motor neuron axons. Primary motor neurons from the 18 somite stage of zebrafish embryos were isolated. Neurite outgrowth could be rescued by supplying carbachol, a cholinergic agonist. However, atropine (a muscarinic receptor) application in atcay,acl and chat knock-downs inhibited neurite outgrowth in vitro , this phenotype was not rescued by carbachol. These data confirm that atcay functions through muscarinic acetylcholine receptors and the MAPK (mitogen-activated protein kinase) pathway to regulate neurite outgrowth. The subcellular location of Chat changed in atcay and acl morphants, with Chat Cells 2021,10, 836 16 of 28 optic tecta and cerebellum. Co-injection of rnf216 and otud4 morpholinos produced a more severe cerebellar phenotype, accompanied with an increased reduction in the size of the optic tecta and marked microphthalmia. Co-injection of human RNF216 or OTUD4 mRNA in double morphants rescued the phenotype, but this was not the case for co-injection of mutant RNF216 or OTUD4 mRNA alone. These data suggest that epistatic interactions between these mutations contribute to the disease phenotype [42]. Zebrafish morphants of rnf216 and otud4 showed cerebellar damage characteristic of Gordon Holmes syndrome that should be reproduced in a zebrafish mutant model. The presence of cerebellar abnormalities indicates that these might be interesting models to search for a possible treatment for this syndrome, such as the possibility of performing an unbiased drug screen. • Childhood-onset neurodegeneration with ataxia, dystonia, and gaze palsy (NADGP). Biallelic mutations in the SQSTM1 (sequestosome 1) gene, which is required for intracellular signaling, the oxidative stress response, apoptosis and autophagy, cause NADGP. Dominant mutations in SQSTM1 have been also related with Paget’s disease of the bone, amyotrophic lateral sclerosis and frontotemporal dementia (ALS/FTD) [43]. Knock-down of the sqstm1 gene in zebrafish led to abnormal motor behavior consistent with a reduced touch-evoked escape response. Motor neuron axons were seen to suffer disrupted arborization and shortening. However, there was no neuronal loss or Mauthner cell defects in sqstm1 morphants. Co-injection of human SQSTM1 mRNA rescued the phenotype but this was not rescued by the co-injection of human SQSTM1 mRNA with ALS/FTD mutations. Moreover, overexpression of wild type and mutant human mRNAs did not reproduce the morphant phenotype. As SQSTM1 is known to regulate the activity of mTOR (regulates responses to DNA damage), mTOR levels were measured in sqstm1 morphants and increased levels of mTOR were found. Treatment with rapamycin (an mTOR inhibitor) at 48 hpf resulted in amelioration of the motor phenotype of sqstm1 morphants [97]. In addition, sqstm1 knock-down in a splice site related with cerebellar ataxia, induced structural cerebellar defects in 60% of the embryos which that were specific (as no other phenotypic defects were found). These cerebellar defects ranged from depletion of the axonal connections across the midline of the cerebellum to complete atrophy. These cerebellar phenotypes were rescued by the co-injection of human SQSTM1 mRNA, but not with the co-injection of human SQSTM1 mRNA with disease mutations [43]. The presence of locomotor defects and cerebellar abnormalities make these morpholinos interesting for future studies that compare these findings with new mutant models and to search for treatments that can rescue these specific phenotypes. • Spinocerebellar ataxia autosomal recessive type 7 (SCAR7) and ceroid lipofuscinosis neuronal 2 (CLN2). TPP1 (tripeptidyl peptidase 1) is a serine protease mainly expressed in the lysosome and melanosome. TPP1 mutations have been linked with SCAR7 and CLN2. It has been proposed that loss of function variants with abolished TPP1 enzyme activity leads to CLN2 disease, whereas variants that diminish TPP1 enzyme activity lead to SCAR7 [44]. Morpholino knock-down of tpp1 in zebrafish causes severe developmental defects starting at 28 hpf with an abnormal head and increased apoptosis throughout the body. At 52 hpf, tpp1 morphants developed curly tails and cardiovascular defects such as cardiac loop malformation, pericardial edema, reduced cardiac contractility and low blood flow through the heart [98]. More recently, a knock-out of the tpp1 gene was observed to recapitulate the pathological and behavioral features of CLN2 disease. Tpp1 mutant zebrafish defects started at 48 hpf with a curved body, reduced head and a smaller retina. At 72 hpf, there was no detectable jaw and at later stages the swim bladder was not present in tpp1 mutants. In addition, tpp1 mutants died prematurely before 7 dpf. Stored levels of subunit c of mitochondrial ATP synthase in lysosomes, which is a characteristic of CLN2 disease, were Cells 2021,10, 836 17 of 28 observed to be increased in the whole body including the eye, head, spinal cord, and most prominently, the muscle fibers in 48 hpf tpp1 mutants. CNS examination revealed a deep absence of HuC/D-positive differentiated neurons in the retina, optic tectum and cerebellum of tpp1 mutants and tpp1 morphants. Moreover, astrocytosis was observed in the thalamus and cerebellum of tpp1 mutants at 48 hpf. Selective apoptosis was seen in the retina, optic tectum, cerebellum and spinal cord in tpp1 mutants at 48 hpf. This selective apoptosis is similar to that found in human patients of CLN2 disease. Decreased proliferation was shown at 48 hpf in the retina, forebrain, midbrain–hindbrain boundary and spinal cord of tpp1 mutants and tpp1 morphants. Axonal disorganization, which is another feature of CLN2 disease, was shown to start at 48 hpf in tpp1 mutants and tpp1 morphants. Axonal disorganization in tpp1 deficient zebrafish was characterized by posterior commissure defasciculation, absence of the trochlear nerve and almost complete absence of the optic nerve, which failed to send fibers to the optic tectum. No axonal defects were seen before 48 hpf and primary axon tract formation was not affected in tpp1 deficient models, meaning that axonal loss was secondary to degenerative changes. Locomotion was impaired in tpp1 mutants at 72 hpf. Mutants had an aberrant swimming pattern demonstrating many turns, a significantly increased hyperactive behavior covering long distances, and seemed to show convulsions. At 96 hpf, tpp1 mutants displayed sustained muscle contractions and lost the ability to move. The touch-evoked escape response was also reduced in tpp1 mutants [ 99 ]. Seizure activity in tpp1 mutants was demonstrated through single electrode electroencephalography. Treatment with valproate, but not with pentobarbitone, significantly reduced seizure-related movement and reduced the mortality between 3 and 6 dpf [ 100 ]. This exhaustive research and the positive results obtained with valproate open up the possibility of performing high throughput drug screen against CLN2 in tpp1 zebrafish mutants. •Spinocerebellar ataxia autosomal recessive type 24 (SCAR24). Biallelic mutations in the UBA5 (ubiquitin-activating enzyme of UFM1) gene were recently seen to cause SCAR24 [ 45 ] and early onset encephalopathy with intellectual deficiency, microcephaly, movement disorders, and epilepsy [ 101 ]. Studies in fibroblasts from affected individuals showed that UBA5 mutations impaired the process of UFMylation, resulting in an abnormal endoplasmic reticulum structure [101]. Injection of uba5 morpholinos in zebrafish embryos did not result in a morphological phenotype. However, locomotion defects were observed in these morphants. Uba5 morphants had reduced movements and difficulties to exit the chorion in comparison with wild type larvae. The touch-escape response of uba5 morphant larvae at 72 hpf was decreased. Larvae exhibited looping or pinwheel swimming which resembled a seizure-like behavior. The spontaneous motility of uba5 larvae at 5 dpf was observed to be severely affected [ 101 ]. The next necessary step will be to develop a uba5 zebrafish mutant line to reveal whether it recapitulates the uba5 morpholino locomotion defects. More research is also needed to understand the cellular/molecular/physiological defects caused by uba5 knock-down. •Galloway-Mowat syndrome. Galloway-Mowat syndrome is caused by mutations in the WDR73 (WD repeat domain 73) gene, which has high levels of expression in the brain, mainly in the cerebellum [46]. A Galloway-Mowat syndrome zebrafish model was generated using wdr73 morpholinos. Wdr73 morphants demonstrated a reduced head size, brain morphology defects, hypopigmentation—which displayed incomplete penetrance—and a curved body or truncated tail region at 1–2 dpf. Wdr73 morphants lacked expression of dmbx1a, which is related to midbrain progenitor cells, in the cerebellum at 48 hpf but not at 24 hpf. At 48 hpf, wdr73 morphants had a poorly expanded and differentiated midbrain. However, fgf8 (fibroblast growth factor 8) expression, which is a marker of progenitor cells of the midbrain-hindbrain boundary, was equal to that of wild type embryos. Morphogenesis of the midbrain and hindbrain was disrupted in wdr73 morphants, leading to dilated ventricles. Proliferation of progenitor cells was also reduced in wdr73 morphants at 1 dpf. Purkinje cells in wdr73 Cells 2021,10, 836 18 of 28 morphants were absent at 4 dpf. This cerebellar phenotype was rescued in all the larvae co-injected with zebrafish wdr73 mRNA and in the majority of larvae co-injected with human WDR73 mRNA. In contrast, co-injection with human mRNA containing a nonsense mutation related to Galloway-Mowat syndrome did not rescue the phenotype [ 46 ]. As was previously mentioned for other morpholino models, the creation of mutant lines that recapitulate the cerebellar phenotype is fundamental to progress research in this area, especially when morpholinos cause severe morphological defects such as in this case. •Spinocerebellar ataxia autosomal recessive type 12 (SCAR12). SCAR12 is produced by mutations in the WWOX (WW domain containing oxidoreductase) gene, which has functions in DNA repair and acts as tumor suppressor gene [ 48 ]. Tsuruwaka and colleagues used morpholinos and siRNA to knock-down zebrafish wwox to study intracellular Ca 2+ dynamics. Wwox knock-down caused severe edemas, curled backbones, reduced body length, head and eye size and increased lethality in embryos. In addition, these models had altered Ca 2+ dynamics [ 102 ]. This model presented developmental delay, which is a characteristic of SCAR12 and also had disturbed Ca 2+ dynamics, which remarks the wwox role in DNA repair. However, the CNS was not studied and locomotion assays to evaluate epilepsy were not performed. Future studies looking at these aspects will inform us as to whether zebrafish can be a good model for SCAR12. 3.3. Recessive Inherited Disorders Related to Ataxia In this section we discuss several zebrafish models designed to model pathologies that present ataxia as one of their symptoms: Niemann–Pick disease type C (NPC), CAMRQ3, Joubert syndrome and pontocerebellar hypoplasia. •Niemann–Pick disease type C (NPC). NPC is a rare neurodegenerative lysosomal storage disorder caused by mutations in the NPC1 (95% of the cases) or NPC2 genes, which are involved in cholesterol trafficking. The clinical diagnosis requires fibroblast staining with filipin to determine whether accumulation of unesterified cholesterol in lysosomes is present [50]. Morpholino knock-down of npc1 in zebrafish led to developmental delay characterized by a reduced progression of epiboly. Co-injection with Npc1 mouse mRNA rescued the epiboly delay. When the npc1 morpholino was injected in the yolk syncytial layer at 1000 cell stage, epiboly was delayed more often. This means that npc1, expressed in the yolk syncytial layer, is critical for normal epiboly movements. Analysis of mesoderm induction and cell fates revealed that both develop normally in npc1 morphants. Actin cytoskeleton disorganization was also observed in npc1 morphants, with actin clumping in some cells and localized loss of actin microfilaments in other cells. Treatment with the steroid hormones pregnenolone and Dex in npc1 morphants partially rescued epiboly delay and actin cytoskeleton defects, suggesting that a reduction in steroidogenesis was, in part, responsible for the epiboly delay phenotype in npc1 morphants. Npc1 morphants that completed epiboly presented a phenotype characterized by shorter body axis, wider notochord and somites and died before 2 dpf. Apoptosis increased in npc1 morphants at 1 dpf. In addition, npc1 morphants displayed punctate sterol distribution in cells after filipin staining at 12 hpf [103]. Since thrombocytopenia is found in some patients with NPC1, this symptom was also studied by Louwette et al. [ 104 ] in npc1 morphants. Zebrafish injected with npc1 morpholinos had malformed heads and dysmorphic brains and eyes. Filipin staining revealed defective intracellular processing of cholesterol. Study of thrombocytes revealed that, even with a low dose of morpholino, 82% of the embryos had an almost complete absence of thrombocytes in the caudal hematopoietic tissue at 3 dpf. When the dose was doubled, 90% of the embryos had thrombocytopenia and died at 5 dpf. Erythrocytes numbers were significantly reduced in npc1 morphants [104]. The generation of a npc1 stable mutant model using CRISPR/Cas9 was able to reproduce some of the symptoms of human patients. Npc1 mutant zebrafish had a reduced Cells 2021,10, 836 19 of 28 lifespan; the majority of them died before 2 months post-fertilization and none of them survived after 8 months. Moreover, npc1 mutants had a reduced body length and exhibited ataxia symptoms. Histological analyses allowed for the observation of macroscopic hepatomegaly and splenomegaly with foamy and vacuolated liver cells. Lipid accumulation in the livers of npc1 mutants and a massive accumulation of cholesterol in hepatocytes was also observed. A lipid profile analysis of liver tissues revealed significant differences in npc1 mutants in profiles of ceramide, diacylglycerol, lysophosphatidic acid, phosphatidic acid, phosphatidylcholine, phosphatidyl ethanolamine, phosphatidyl serine and triglyceride, as compared to wild types. Interestingly, seven ceramides—which are characteristic of NPC1 disease—were accumulated in the liver of npc1 mutants. Finally, calretinin expression was significantly reduced in the cerebellum of npc1 mutants at two months post-fertilization, which indicates a loss of Purkinje cells [105]. Tseng et al. [ 106 ] also generated a CRISPR/Cas9 npc1 model that had reduced lifespan (died before 6 months of age), infertility and reduced body length compared to wild type fish. Moreover, adult npc1 mutants failed to maintain balance during swimming and died a few days after the balance defect was observed. Histopathological analyses revealed axonal spheroids in the hindbrain of adult npc1 mutants and disorganized Purkinje neurons in the cerebellum. The first sign of liver disease appeared at 7 dpf in npc1 mutants. They had bigger, dark and opaque livers as compared to wild type larvae. Histopathological analysis of liver sections showed larger hepatocytes full of vacuole like structures in npc1 mutants. In addition, filipin staining demonstrated cholesterol accumulation in npc1 mutant liver tissue. Surprisingly, lipid accumulation was not observed in npc1 mutants. Filipin positive staining started at 2 dpf in npc1 mutants in the yolk area and at 3 dpf in lateral line tissues. By 5 and 7 dpf, npc1 mutants accumulated more unesterified cholesterol throughout the entire trunk area. Cholesterol accumulation was observed along the notochord and the ventral edge of the trunk in npc1 mutants. Application of a pCS2+ plasmid with npc1 cDNA and EGFP rescued the unesterified cholesterol accumulation in the yolk area. Lysosomes in live larval zebrafish were observed using LysoTracker Red staining. At 5 dpf, Npc1 mutants had a stronger LysoTracker Red staining signal compared to wild type larvae, mainly in the neuromasts and in the olfactory placode of npc1 mutants at 3 dpf. Based on these results, LysoTracker Red staining was used to test drug efficacy in vivo . The 2HP β CD compound, which was seen to be effective in other animal models and had been tested in humans, was tested on 3 dpf larvae. After 3 days of treatment, a significant reduction in LysoTracker Red staining was observed in npc1 mutants. Filipin staining also revealed reduced accumulation of cholesterol in npc1 mutants. However, the 2HP β CD treatment did not rescue the liver defects or improve survival [ 106 ]. In any case, the development of a method to test compounds in npc1 mutant zebrafish is crucial for attempting to discover new therapies for NPC. • Cerebellar ataxia and mental retardation with or without quadrupedal locomotion 3 (CAMRQ3). Mutations in carbonic anhydrase 8 (CA8) are related to CAMRQ3 [ 51 ]. CA8 is a catalytically inactive isoform belonging to the zinc-containing metalloenzymes family, that catalyzes the reversible hydration of carbon dioxide [52]. The ca8 gene was found to be strongly expressed in the zebrafish nervous system, and specifically, in the Purkinje cells, which correlates with the observed expression in Purkinje cells in humans and mice. Ca8 morpholinos caused defects in the zebrafish head as early as 9 hpf and increased mortality. At 1 dpf, ca8 morphants had defects in the head, a fragile body, curved tail, small eye size and pericardial edema that were dosedependent [ 52 , 107 ]. As development advanced, defects such as the shortened tail, curved body axis, absence of swim bladder became more obvious. The swimming pattern was altered even with a low morpholino dose. Ca8 morphants swam at a slower speed, showed an increased turning angle, and most of them swam along the periphery of the Petri dish. Furthermore, ca8 morphants had a pronounced difficulty in balancing the body while swimming compared with wild type. When the concentration of ca8 morpholino was Cells 2021,10, 836 20 of 28 increased, the larvae progressively lost their ability to swim, until higher doses caused a complete loss. The co-injection of a p53 morpholino did not rescue the phenotype defects or mortality rates. Gross morphological changes in the cerebellar region and a reduction in the size of the cerebellum was observed in ca8 morphants. Moreover, ca8 morphants showed abnormal muscle development and apoptosis in the head region and periphery of the tail region [ 52 ]. Touch-evoked responsiveness was also reduced in ca8 morphants due to defective cerebellar function, as no defects were observed in the motor neurons or Rohon Beard sensory neurons [ 107 ]. Ca8 zebrafish morphants seem to reproduce the typical features observed in CAMRQ3. As with other disorders, it would be of interest to develop a stable zebrafish mutant model that reproduces these (or similar) phenotypes. •Joubert syndrome. Joubert syndrome consists of a group of early onset recessive or X-linked cerebellar ataxias with a characteristic mid-hindbrain malformation called the molar tooth sign [ 53 ]. More than 30 genes have been associated with Joubert syndrome. Several zebrafish models have been created to study some of these genes, but most of them were focused solely on their function in ciliogenesis or retinal development [108–114]. Mutations in the AHI1 (Abelson helper integration site 1) gene are the most common cause of Joubert syndrome. Knock-down of ahi1 in zebrafish caused a curved body and abnormalities in the development of the eye, hindbrain (hydrocephalus) and otoliths, together with defects in cyst formation in the pronephric kidney tubules. These malformations were comparable to those of patients with Joubert syndrome. Co-injection of murine Ahi1 mRNA efficiently rescued the phenotype. Histological analyses revealed defects in lamination of the cell layers of the retina in ahi1 morphants. Reversed cardiac looping with the heart in a L-loop pattern was found in ahi1 morphants. Moreover, cloacal dilatation and loss of pronephric cilia was observed in the pronephric ducts [115]. More recently, Lessieur et al. [ 116 ] generated an ahi1 TALEN mutant model and showed that mutants had cone degeneration and rhodopsin mislocalization in rods at 5 months of age as well as absence of distal pronephric duct cilia [ 116 ]. Zhu et al. [ 117 ] used zebrafish morpholinos and CRISPR/Cas9 mutants to analyze if ahi1 mutations lacking the intact WD40 repeats affect axonal decussation. They found that ahi1 morphants and mutants had retinal ganglion cell axon misprojection and ocular dysplasia caused by a toxic gain of function [117]. Other zebrafish models of different genes related to Joubert syndrome, such as a knock-down model of cep290 (centrosomal protein 290), also recapitulate features of Joubert syndrome, such as cerebellar abnormalities, hydrocephalus, retinal defects, abnormalities in otic cavity development and pronephric cysts [ 118 , 119 ]. Moreover, cep290 morphants were used to search for therapies for ciliopathic renal disease, which resulted in the discovery that rapamycin and roscovitine ameliorate the symptoms [ 120 ]. More recently, a mutant line was developed to study retinal degeneration. Cep290 mutants presented scoliosis and progressive cone deterioration [114]. Similarly, knock-down of cspp1 (centrosome and spindle pole associated protein 1), cep104 (centrosomal protein 104), kiaa0556 (katanin interacting protein) and poc1b (proteome of the centriole 1B) in zebrafish resulted in a ciliopathy phenotype, which is characteristic of Joubert syndrome [121–126]. Most of these Joubert syndrome zebrafish models were not used to study the CNS. In addition, most of them were not created with mutants that we suspect would probably reproduce better the traits of this syndrome. •Pontocerebellar hypoplasia. Pontocerebellar hypoplasia constitutes a group of early onset rare neurodegenerative disorders with variable symptoms of cerebellar ataxia. Several mutations in different genes have been associated with different forms of pontocerebellar hypoplasia. Mutations in TSEN54, a tRNA splicing endonuclease subunit gene, were associated with pontocerebellar hypoplasia type 6 and late onset dominant hereditary ataxia [54]. Cells 2021,10, 836 21 of 28 Morpholino knock-down of tsen54 in zebrafish resulted in brain hypoplasia and loss of structural integrity inside the brain with an aberrant mid-hindbrain boundary. Co-injection of human TSEN54 mRNA partially rescued the brain phenotype. Co-injected embryos displayed milder brain hypoplasia and a more defined brain structure. Interestingly, tsen54 morpholino abnormalities were not associated with neurodevelopmental patterning defects since expression of fgf8 (which plays a role in the maintenance and development of the mid-hindbrain boundary) and otx2 (orthodenticle homeobox 2) (which functions in the early regionalization of the mesencephalon) at 24 hpf was normal. Tsen54 morphants had increased levels of apoptosis in the brain. A stable tsen54 knock-out model created with ENU mutagenesis had a reduced survival rate with all the tsen54 homozygous larvae dying before 9 dpf. However, the defects that caused their lethality were not studied and it is not known if mutations in tsen54 also caused brain hypoplasia. In addition, knock-down of the rars2 (arginyl-tRNA synthetase 2) gene, which has been also related to pontocerebellar hypoplasia type 6, resulted in a similar brain phenotype to that observed in tsen54 morphants, which was also partially rescued by the co-injection of RARS2 human mRNA [ 127 ]. The better characterization of the mutant model would help to study the molecular consequences of pontocerebellar hypoplasia. Mutations in the SLC25A46 (solute carrier family 25 member 46) gene, which plays a role in mitochondrial dynamics, have been also related to pontocerebellar hypoplasia and progressive myoclonic ataxia with optic atrophy and neuropathy [128,129]. Slc25a46 was observed to be prominently expressed in the brain and the spinal cord during zebrafish embryonic development. Consistent with this, slc25a46 zebrafish morphants showed a neurodegenerative phenotype with a failure of the development of the midbrain and hindbrain, severe curly tail morphology and abnormal locomotion. Motor neurons had significantly shorter axon tracts and many of them failed to innervate the rostral myotome at 48 hpf, the spinal cord neuropil had fewer neuronal processes, fewer retinal ganglion cell axons reached the tectum at 72 hpf, and retinal ganglion cell dendrites were also affected. Degeneration of motor neuron terminals was also observed. Slc25a46 zebrafish morphants presented a misallocation of the mitochondria, which were in the process of fission within the cell bodies. This suggested that incomplete fission of mitochondria in slc25a46 morphants might inhibit transport and distribution into neuronal processes. Mitochondrial dynamics were studied in dissociated neurons from slc25a46 zebrafish morphants. Mitochondria from morphants were longer than those of wild type embryos and were immobile. Co-injection with SLC25A46 human mRNA restored the size of the mitochondria but not the co-injection with mutant SLC25A46 mRNA. On the other hand, overexpression of the wild type mRNA resulted in mitochondrial fragmentation and disruption of the mitochondrial network [129,130]. In contrast to the morphant studies, a CRISPR/Cas9 slc25a46 zebrafish model showed no phenotype because of genetic compensation, as was demonstrated by RNA sequencing. Injection of a slc25a46 morpholino into an F2 homozygous slc25a46 zebrafish CRISPR/Cas9 line did not cause a phenotype. However, F0 embryos injected with an slc25a46 CRISPR/Cas9 construct had a phenotype that resembled slc25a46 morphants since they had smaller eyes, heart edema, a shorter trunk and an increase in motor neuron axon disruptions in comparison with wild types. The F0 slc25a46 CRISPR/Cas9 phenotype was rescued after the co-injection of SLC25A46 human mRNA. The existence of a phenotype in slc25a46 CRISPR/Cas9 mosaics of the F0 generation, but not in the homozygous F2 generation, indicates that the genetic compensation starts after the F0 generation. RNA sequencing showed a high number of serine proteases and their transcription factors, serine protease inhibitors, DNA-binding proteins and a smaller number of transporters, proteins related to immunity that were expressed differentially in F2 slc25a46 CRISPR/Cas9 embryos at 48 hpf [ 131 ]. In this case, it seems that the slc25a46 morphant model better represents the main features of pontocerebellar hypoplasia caused by mutations in SLC25A46 (and not the mutant homozygous model that suffers genetic compensation). This morphant model will help to further study pontocerebellar hypoplasia and search for possible treatments. Cells 2021,10, 836 22 of 28 4. Conclusions The majority of the zebrafish models discussed here for genes related with recessive ataxias reproduced some of the neuronal and non-neuronal phenotypes observed in human disorders. The models that did not develop any neuronal symptoms or locomotor deficits were: atm morphants and mutants [ 55 , 56 ]; polg mutants [ 89 , 90 ]; ptf1a morphants, mutants and transgenic lines [ 91 – 96 ]; wwox morphants and siRNA models [ 102 ]. In any case, atm models developed other non-neuronal symptoms of AT such as radiosensitivity, infertility and immunodeficiency [ 55 , 56 ]. Polg mutants, which were analyzed in order to study mitochondrial disease, showed reduced mitochondrial numbers, reduced respiratory levels in the CNS, and altered locomotion [ 89 , 90 ]. ptf1a models reproduced the pancreatic agenesis of PACA [ 91 – 96 ]. wwox knock-down models, which demonstrated developmental delay, were only used to study Ca 2+ dynamics, highlighting the role of wwox in DNA repair [ 102 ]. In addition, snx14 mutants [ 61 ] did not recapitulate the snx14 morphant motor neuron deficit phenotype [27], but revealed a role for this gene in lipid biogenesis [61]. Most of the publications of autosomal recessive ataxias employed morpholinos to cause a knock-down and a loss of function effect. The morpholino effect is transient, its degradation occurs in few days and can sometimes cause off-target effects. For this reason, it is fundamental to validate it with morpholino controls (standard or mismatch morpholinos), PCR/Western blot/immunohistochemistry and mRNA rescue. As stated above for several models, stable mutant lines are necessary to complement morpholino studies because they are more informative and might facilitate drug screening [ 62 ]. However, mutant models do not always recapitulate the phenotypes observed with morphants due to genetic compensation and maternal mRNA rescue. Although zebrafish are not expected to fully reproduce the human phenotypes due to their less intricate CNS and their limited number of complex behaviors, they are very informative for unravelling gene functions and analyzing gene and molecular pathways. In addition, their small size and external fertilization simplify high throughput drug or genetic screening. In this review, we reported various drug treatments that alleviate the symptoms of zebrafish models of autosomal recessive ataxias [ 70 , 79 , 90 , 97 , 100 , 103 , 106 , 120 ]. Future work should apply the use of these models for high throughput drug screening. Recent technological advances in genetic editing, such as the development of CRISPR/Cas technologies [ 132 ], will improve the number of specific stable mutant lines that better mimic human conditions, while the use of novel techniques of microscopy and imaging, such as super-resolution or light-sheet microscopy, in zebrafish will ease phenotypic characterization. Supplementary Materials: The following are available online at https://www.mdpi.com/article/ 10.3390/cells10040836/s1, Supplementary Table S1: Description of zebrafish models of autosomal recessive ataxias. Author Contributions: Writing—original draft and figure preparation, A.Q.-R.; writing—review and editing, D.S.-C., A.B.-I., M.J.S. and L.S. All authors have read and agreed to the published version of the manuscript. Funding: This research was funded by Fondo de Investigaciones Sanitarias-Instituto de Salud Carlos III (Spain), grant number: PI17/01582 and by the Asociación Galega de Ataxia (AGA). Conflicts of Interest: The authors declare no conflict of interest. References 1. Evidente, V.G.; Gwinn-Hardy, K.A.; Caviness, J.N.; Gilman, S. Hereditary Ataxias. Mayo Clin. Proc. 2000 ,75, 475–490. [CrossRef] 2. Beaudin, M.; Klein, C.J.; Rouleau, G.A.; Dupré, N. Systematic Review of Autosomal Recessive Ataxias and Proposal for a Classification. Cerebellum Ataxias 2017,4, 3. [CrossRef] 3. Beaudin, M.; Matilla-Dueñas, A.; Soong, B.-W.; Pedroso, J.L.; Barsottini, O.G.; Mitoma, H.; Tsuji, S.; Schmahmann, J.D.; Manto, M.; Rouleau, G.A.; et al. 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