Next Article in Journal
Genomic Analysis Defines Increased Circulating, Leukemia-Induced Macrophages That Promote Immune Suppression in Mouse Models of FGFR1-Driven Leukemogenesis
Previous Article in Journal
Multi-Fused S,N-Heterocyclic Compounds for Targeting α-Synuclein Aggregates
 
 
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Article

Conditional ATXN2L-Null in Adult Frontal Cortex CamK2a+ Neurons Does Not Cause Cell Death but Restricts Spontaneous Mobility and Affects the Alternative Splicing Pathway

1
Clinic of Neurology, Experimental Neurology, University Hospital, Goethe University Frankfurt, Heinrich-Hoffmann-Str. 7, 60528 Frankfurt am Main, Germany
2
Institute for Clinical Neuroanatomy, Dr. Senckenberg Anatomy, Fachbereich Medizin, Goethe University Frankfurt, 60528 Frankfurt am Main, Germany
3
Max Planck Institute for Molecular Genetics, Ihnestraße 63-73, 14195 Berlin, Germany
*
Author to whom correspondence should be addressed.
These authors contributed equally to this work.
Cells 2025, 14(19), 1532; https://doi.org/10.3390/cells14191532
Submission received: 8 September 2025 / Revised: 26 September 2025 / Accepted: 28 September 2025 / Published: 30 September 2025

Abstract

Highlights

What are the main findings?
  • Constitutive knock-out of ATXN2L across LSMAD and PAM2 is embryonically lethal, confirming its essential role in development.
  • Conditional deletion of ATXN2L across LSMAD and PAM2 postnatally in cortical neurons reduces spontaneous movement and alters alternative splicing pathways.
What are the implications of the main findings?
  • ATXN2L is indispensable for embryonic survival and neuronal function, highlighting its non-redundant role, in contrast to its paralog ATXN2.
  • The LSMAD and PAM2 domains of ATXN2L likely impact nuclear splicing, despite the protein’s perinuclear localization.

Abstract

The Ataxin-2-like (ATXN2L) protein is required to survive embryonic development, as documented in mice with the constitutive absence of the ATXN2L Lsm, LsmAD, and PAM2 domains due to knock-out (KO) of exons 5–8 with a frameshift. Its less abundant paralog, Ataxin-2 (ATXN2), has an extended N-terminus, where a polyglutamine domain is prone to expansions, mediating vulnerability to the polygenic adult motor neuron disease ALS (Amyotrophic Lateral Sclerosis) or causing the monogenic neurodegenerative processes of Spinocerebellar Ataxia Type 2 (SCA2), depending on larger mutation sizes. Here, we elucidated the physiological function of ATXN2L by deleting the LsmAD and PAM2 motifs via loxP-mediated KO of exons 10–17 with a frameshift. Crossing heterozygous floxed mice with constitutive Cre-deleter animals confirmed embryonic lethality among offspring. Crossing with CamK2a-CreERT2 mice and injecting tamoxifen for conditional deletion achieved chimeric ATXN2L absence in CamK2a-positive frontal cortex neurons and reduced spontaneous horizontal movement. Global proteome profiling of frontal cortex homogenate showed ATXN2L levels decreased to 75% and dysregulations enriched in the alternative splicing pathway. Nuclear proteins with Sm domains are critical to performing splicing; therefore, our data suggest that the Like-Sm (Lsm, LsmAD) domains in ATXN2L serve a role in splice regulation, despite their perinuclear location.

1. Introduction

The Sm domain is an ancient RNA-binding motif with oligo(U) specificity that assembles into heteroheptameric rings [1], with similarity to nuclear Sm core ribonucleoprotein rings in the spliceosome and to cytosolic Like-Sm (LSm) ribonucleoprotein rings that mediate mRNA decapping and decay [2]. In bacteria and archaea, the Sm domains in Hfq homologs have been extensively studied to characterize their best-known role in intron splicing from pre-mRNA and to demonstrate their functions as chaperones that mediate interactions between regulatory non-coding RNAs and their targets, as well as functions for the maturation of tRNAs/rRNAs [3].
With the evolution of multi-domain proteins in eukaryotic cells, RNA processing has become more efficient, particularly with the discovery of a cytoplasmic ribonucleoprotein family with a length of 600 to 1000 amino acids (exemplified by the Saccharomyces cerevisiae yeast protein Pbp1), which provides binding sites for (i) RNA in the Lsm domain, (ii) RNA helicases in the area from Lsm to Lsm-associated domain (LsmAD) sequences, and (iii) poly(A)-binding proteins at the PAM2 motif. In cellular stress periods, Pbp1 and all its orthologs relocalize away from the translation apparatus to stress granules, where RNA quality control and triage are performed [4,5,6,7]. Other currently studied family members include ATX-2 in Caenorhabditis elegans worms [8,9,10,11,12,13], dATX2 in Drosophila melanogaster flies [14,15,16,17,18,19,20,21,22,23,24,25,26,27,28], and ATXN2 in Gallus gallus birds [29]. With increasing organism mass, and outside the temperate sea environment, gene duplication has been conserved from ray-finned fish to mammals. The less abundant—but N-terminally much extended—version with around 1300 amino acids is called Ataxin-2 or hATXN2 in humans; conversely, a relatively unchanged and more abundant version with around 1000 amino acids is known as Ataxin-2-like or ATXN2L. Furthermore, land plants carry two gene copies (known in Arabidopsis thaliana as CID3/CID4) [30].
Research on patients with autosomal-dominant, chronically progressive spinocerebellar ataxia type 2 (SCA2) has identified unstable expansions in the polyglutamine (polyQ) domain, surrounded by Proline-rich motifs (PRM) in the N-terminus of hATXN2, as a cause of disease [31,32,33]. This has provided a name for this gene family and initial insights into its physiological and pathological roles [10,34,35,36,37,38,39,40,41,42,43,44,45,46,47,48,49,50,51,52,53]. Subsequent findings show that this gene modifies the risk and disease progression of adult motor neuron degenerations such as Amyotrophic Lateral Sclerosis (ALS) [54,55,56,57,58]. This has intensified analyses of its impact on RNA maturation and RNA quality control in stress granules [15,18,19,22,25,28,59,60,61,62,63,64,65,66,67,68,69,70]. Mammalian ATXN2 appears to mediate rapid stress responses and increase fitness, but its deletion results in obesity, hepatosteatosis, hyperinsulinemia, and hypercholesterolemia [39,48]; however, its excessive gain-of-function restricts nutrient endocytosis, represses mTORC1-dependent growth, decreases cholesterol biosynthesis, and depletes myelin lipids [41,50,66,71]. Interestingly, the precise circadian clock rhythms are regulated by oscillating waves of translation, where ATXN2 depletion triggers an advanced phase shift, whereas ATXN2L depletion triggers a delayed phase shift [68]; therefore, the function of these two ribonucleoproteins may be complementary or antagonistic.
Pathogenic mutations in patients have not been documented for ATXN2L, and only very few studies have been dedicated to mammalian ATXN2L. It conserves the classical domain combination Lsm-LsmAD-PAM2 but has a PRM and MPL binding region at its N-terminus [72] and an additional Pat1 homology sequence at its C-terminus (which is absent from ATXN2 [62]). Pat1 proteins usually interact with the cytosolic Lsm1-7 ring to promote deadenylation-dependent decapping and degradation of 3′ UTR AU-rich mRNAs in P-bodies [73,74,75,76]; however, they can undergo nuclear relocation to Cajal bodies/speckles upon stress and interact with nuclear Lsm2-8 rings complexed with U6 snRNA to promote splicing [77,78,79], with a prominent role in the growth of synaptic terminals [80]. ATXN2L can localize to nuclear splicing speckles [62], and its nuclear localization depends on its PRMT1-dependent arginine methylation [81]. Its normally cytosolic distribution shows more of a perinuclear concentration than ATXN2 [82]. Upon constitutive knock-out of Atxn2l exons 5–8 with a subsequent frameshift in the mice, their homozygous offspring suffered from mid-gestational embryonic lethality, with brain neuronal lamination defects and apoptosis [83]. In proteome profiles of murine embryonic fibroblasts, ATXN2L loss results in similarly strong deficits in RNA processing factor NUFIP2 and nuclear envelope factor SYNE2; both proteins are interactors of ATXN2L [82], but it remains unclear which protein dysregulations mediate the preferential ATXN2L impact on neural tissue.
To obtain an initial understanding of ATXN2L deficiency’s impact on adult neurons at the behavioral, cellular, and molecular levels, we generated the first mouse line with floxed Atxn2l for conditional manipulations, where an N-terminal fragment of ATXN2L with the Lsm domain may still exist, but the remaining protein is ablated.

2. Materials and Methods

2.1. Mouse Breeding and Genotyping

All animal experiments complied with the German Animal Welfare Act, European Directive 86/609/EWG (24 November 1986, Annex II), and the ETS123 guidelines (European Convention for the Protection of Vertebrate Animals). Mice were maintained in the Central Animal Facility (ZFE) of the Goethe University Medical School under standard conditions: individually ventilated cages containing nesting material, a 12 h light–12 h dark cycle, controlled temperature and humidity, and free access to food and water. Colony maintenance and expansion were achieved by breeding heterozygous carriers. For experimental comparisons, sex-matched mutant and wild-type (WT) littermates were housed together. Both male and female animals were included in all experiments. Ethical approval was obtained from the Regierungspräsidium Darmstadt (permit number V54-19c20/15-FK/2032). The analysis of Ataxin-2-like isoforms and the subsequent development of an Atxn2l conditional knock-out (cKO) mouse line in the C57BL/6 genetic background via homologous recombination were outsourced to the Genoway company (Lyon, France). The targeting vector was designed using sequences from Mus musculus strain C57BL/6J chromosome 7, GRCm39, NC_000073.7, nucleotide positions 126075978 to 126115977. Sperm from the successfully floxed Atxn2l mice were deposited at Genoway. SnapGene (Boston, MA, USA, Version 8.0.2) was used for structural analysis and primer generation.
To trigger the Atxn2l-KO constitutively, mice with targeted flox site insertion were bred with pan-Cre-deleter mice to obtain heterozygous Atxn2l-KO mice for intercrosses. To selectively trigger the Atxn2l-cKO in CamK2a-positive cells, homozygous Atxn2l-flox mice were crossed with CamK2a-Cre/ERT2 mice (B6;129S6-Tg(CamK2a-Cre/ERT2)1Aibs/J, Jackson Laboratories, Bar Harbor, Maine, USA). Resulting double mutants that were heterozygous for Atxn2l-flox and expressed Cre recombinase (Atxn2l-WT/flox, CamK2a-Cre/ERT2-Tg) were then crossed with homozygous Atxn2l-flox mice to generate homozygous Atxn2l-flox mice with transgenic Cre (Cre-Tg). Homozygous Atxn2l-flox mice without Cre served as littermate controls. All genotyping primers are provided in Table S1.
To genotype the floxed Atxn2l, DNA from ear tissues was extracted using the hot shot method [84], performing the PCR with 1 µL of DNA in a reaction mix with AmpliTaq (Thermo Fisher, Waltham, MA, USA). The PCR conditions were 3 min at 94 °C; 35 cycles of 30 s at 94 °C, 30 s at 65 °C, and 30 s at 72 °C; followed by 5 min at 72 °C. The expected bands were 315 bp for the WT allele and 405 bp for the floxed allele.
To genotype the Cre transgene, a touchdown PCR was performed, as recommended by the Jackson website (https://www.jax.org/Protocol?stockNumber=012362&protocolID=27167, last accessed on 6 June 2024). Then, 5 min at 94 °C was followed by 10 cycles with a decrease of 0.5 °C per cycle with 30 s at 94 °C, 30 s at 65 °C, and 30 s at 68 °C. This was followed by 28 cycles of 30 s at 94 °C, 30 s at 60 °C, and 30 s at 72 °C, with 7 min at 72 °C at the end. The expected band sizes were 521 bp for the control and 200 bp for the presence of Cre.
To genotype the Atxn2l-KO, the PCR conditions were 3 min at 94 °C; 35 cycles of 30 s at 94 °C, 30 s at 66 °C, and 30 s at 72 °C; followed by 5 min at 72 °C. The expected bands were 151 and 3808 bp for the WT allele and 276 bp for the KO allele.

2.2. Assessment of Embryonic Lethality in Constitutive Atxn2l-KO Mice

After excision of the neo cassette and the floxed region in vivo, 2 heterozygous mice with constitutive deletion of Atxn2l exons 10–17 were obtained, which were then crossed with C57BL/6 mice to generate a colony. Multiple breeding units of male and female heterozygotes were used to analyze the offspring for the viability of Atxn2l-KO mice and the distribution of heterozygous versus WT animals among the offspring. In total, 100 litter pups were produced and genotyped.

2.3. Immunohistochemistry

Serial frontal sections of 50 µm thickness were cut using a vibratome (Leica VT 1000 S Leica, Wetzler, Germany) and collected in PBS. Individual sections were incubated in a blocking solution (10% normal goat serum (NGS), 0.5% Triton X-100 in PBS) at RT for 2 h. Afterward, sections were incubated overnight at RT in primary antibodies (rabbit-anti-ATXN2L, 1:300, Proteintech Cat# 24822-1-AP, RRID: AB_2879743; mouse-anti-CAMK2a, 1:500, Santa Cruz Biotechnology Cat# sc-70492, RRID: AB_1119957) diluted in antibody solution (5% NGS, 0.2% Triton X-100 in PBS). Sections were washed three times (PBS, 10 min each) and then incubated in the dark for 2 h at room temperature with secondary antibodies diluted in antibody solution (goat-anti-rabbit Alexa Fluor 568, 1:1000, Thermo Fisher Scientific Cat# A-11036, RRID: AB_10563566; goat-anti-mouse Alexa Fluor 488, 1:1000, Thermo Fisher Scientific Cat# A-11029, RRID: AB_2534088). Sections were then washed three times in PBS for 10 min, with the second wash containing the nuclear stain Hoechst (1:5000). Finally, sections were mounted on glass slides with mounting medium (Dako/Agilent, Santa Clara, CA, USA).

2.4. Imaging

Fluorescent widefield overview images were acquired with an IXplore Live IX83 LED (Evident) using a 4× objective (UPlanXApo, NA 0.16, Thermo Scientific, Waltham, MA, USA). Higher-magnification images were acquired with a Nikon C2si laser scanning confocal microscope (Nikon, Amstelveen, The Netherlands) equipped with a 20× objective (Plan Apo, NA 0.75, Thermo Scientific, Waltham, MA, USA) at a resolution of 1024 × 1024 pixels, using a 2× average. Images of control and cKO brains were acquired with equal exposure times/laser and gain settings. Brightness and contrast of the overview images in Figure 3A were post hoc-adjusted in FIJI [85] (RRID: SCR_002285) for visualization purposes; adjustments were equally applied to control and cKO images.

2.5. Locomotor Phenotyping

Assessment of spontaneous movements was performed in an open field apparatus (Versamax, Omnitech, Columbus, OH, USA), simultaneously placing tamoxifen-treated Atxn2l-flox versus Atxn2l-flox/Cre mice at monthly intervals into 20 × 20 cm chambers, recording their activity using infra-red beams during 5 min trials, and interrogating predefined parameters for alterations with consistency over time, as previously described [61]. Atxn2l-flox/Cre-Tg animals were injected with TAM to induce the conditional KO (Atxn2l-cKO), in parallel with Atxn2l-flox mice that lacked Cre and served as controls (Atxn2l-flox/Cre-WT).

2.6. Tamoxifen Preparation and Treatment

A tamoxifen solution (20 mg/mL) was prepared from 200 mg of tamoxifen powder (Sigma-Aldrich #T5648, Burlington, MA, USA) and reconstituted in 10 mL of peanut oil (Sigma-Aldrich #P2144, USA). Tamoxifen was dissolved directly in peanut oil at room temperature with vertical rotation overnight and subsequent vortexing. Mice were weighed before the first injection, and the volume to be injected was calculated for a tamoxifen dose of 75 mg/kg body weight. Intraperitoneal tamoxifen injections were applied on five consecutive days, using 0.3 mL syringes and 30-gauge × 8 mm needles (Becton, Dickinson and Co. #324826, Franklin Lakes, NJ, USA).

2.7. Global Proteomics

Mice were euthanized through cervical dislocation, after which the brains were dissected, snap-frozen in liquid nitrogen, stored at −80 °C, and transported on dry ice. For proteomic analysis, eight left frontal cortex specimens (4 Atxn2l-cKO and 4 Atxn2l-flox/Cre-WT) were included. This sample number was chosen to allow for the exclusion of one potential mis-genotyped animal or outlier per group while still maintaining sufficient power to detect major effects. To uncover more subtle changes in future experiments, the use of a non-mosaic Cre driver line is advisable.
Tissues were homogenized in denaturing buffer using a FastPrep system (1 × 60 s, 4.5 m/s) in 800 µL of freshly prepared buffer (3 M guanidinium chloride, 10 mM tris(2-carboxyethyl)phosphine, 20 mM chloroacetamide, 100 mM Tris-HCl, pH 8.5). Lysates were heated to 95 °C for 10 min with shaking (1000 rpm, thermal mixer) and subsequently sonicated in a water bath for 10 min. After centrifugation, supernatants were transferred to low-binding 1.5 mL tubes (Eppendorf, Hamburg, Germany). Protein concentrations were quantified by BCA assay (Thermo Scientific, USA; kit no. 23252). Each sample (500 ng) was diluted in buffer containing 10% acetonitrile and 25 mM Tris-HCl, pH 8.0, to reach 1 M guanidinium chloride. Proteins were first digested with LysC (MS-grade, Roche, Basel, Switzerland; enzyme-to-protein ratio, 1:50) for 3.5 h at 37 °C, shaking at 800 rpm. The mixture was then diluted to 0.5 M guanidinium chloride and subjected to overnight tryptic digestion (Roche, 1:50 ratio, MS-grade) at 37 °C with agitation. Peptides were acidified with formic acid (final concentration, 2%) and loaded onto Evotip Pure tips (Evosep, Odense, Denmark) according to the manufacturer’s instructions.
Separation of peptides was performed on an Evosep One LC system using an Aurora Elite C18 column (15 cm × 75 µm ID, 1.7 µm beads; IonOpticks, Victoria, Australia) with the 20-samples-per-day method (Whisper Zoom 20-SPD). The LC was directly coupled to a timsTOF Ultra 2 mass spectrometer (Bruker Daltonics, Bremen, Germany) employing data-independent acquisition with the PASEF workflow. Spectral data were analyzed using Dia-NN (v2.0), searching against an in silico-predicted murine spectral library, with the “match between runs” option enabled. The mass spectrometry data have been deposited at the ProteomeXchange Consortium (http://proteomecentral.proteomexchange.org, accessed on 6 June 2024) via the PRIDE partner repository [86] with the data set identifier PXD064497.

2.8. Proteome Interrogation for Pathway Enrichments

The webserver of STRING version 12 (Search Tool for the Retrieval of Interacting Genes/Proteins) (https://string-db.org/, accessed on 6 June 2024) was employed to assess the proteome profile in an automated manner for any enrichments in protein–protein interactions, Gene Ontology (GO) terms, Reactome and KEGG pathways, subcellular localizations, and protein motifs [87]. In addition, to maximize bioinformatics insights, the three Atxn2l-flox/Cre-WT samples with the highest values and the three Atxn2l-cKO samples with the lowest values for ATXN2L abundance (reduction to 70% of controls) were compared for significant dysregulations in the proteome. The resulting list of proteins was visualized as a volcano plot and studied in STRING regarding ATXN2L-dependent interactomes.

2.9. Statistics and Graphical Presentation

Unpaired Student’s t-tests with Welch’s corrections were used to establish comparisons for continuous variables between homozygous Atxn2l-cKO and floxed WT animals. Mean values and variance as standard error of the means (SEM), as well as linear regression lines, were used for behavior data visualization. GraphPad (Version 10.4.1, for Windows, GraphPad Prism, Boston, MA, USA) was used for all statistical analyses and volcano plot generation. Significance was assumed at p < 0.05 and highlighted with asterisks: * p < 0.05.

3. Results

3.1. Generation of Conditional KO Mice via Floxing Exons 10–17 in the Atxn2l Gene

To bypass the embryonic lethality of the constitutive ATXN2L-null genotype and to achieve ATXN2L absence selectively in neural tissue during adult life, we generated the first Atxn2l-cKO mouse strain. The initial bioinformatic characterization of the murine Atxn2l gene revealed 22 exons (Figure 1A), with ATG initiation codons in exons 1 and 2, stop codons in exon 22, translating into one experimentally validated protein with 1049 amino acids. This also provided protein isoforms containing 1074, 994, or 1043 amino acids (analyzing the database mRNA/protein entries in GenBank BC054483/UniProt Q7TQH0-1, GenBank AK155062/UniProt Q7TQH0-2, GenBank AK168745/NCBI NP_001334587, and isoform 4 derived from UniProt entry Q7TQH0-3). The variants showed N-terminal differences regarding the Proline-rich motif (PRM), while the N-terminal potential MPL–interaction region [72] was common to all (Figure 1A). The phylogenetically conserved sequences were always present, including the (i) Lsm domain involved in RNA binding, (ii) the LsmAD sequence (where a clathrin-mediated trans-Golgi signal, an ER exit signal, and a putative caspase cleavage site DxxD were reported), and (iii) the PABP-interaction motif PAM2 involved in mRNA turnover regulation. The ATXN2L variants showed differences at the C-terminus, where sequence homology exists with the Pat1 protein family [62].
To flank Atxn2l exons 10 and 17 with loxP sites, a targeting vector was generated in the mouse C57BL/6 genetic background, thus enabling the selective deletion of a 3.3 kb fragment containing the LsmAD sequence and the PAM2 motif, with a consequent frameshift that eliminates the C-terminal sequences. To drive efficient homologous recombination screens, this vector contained a neomycin-selection cassette with flanking RoxP sites between exons 9 and 10 as a positive selection marker, with murine isogenic Atxn2l genomic sequences comprising a short arm from exon 8 and a long arm extending beyond exon 22, together with diphtheria toxin fragment A as a negative selection marker (Figure 1B). An optimal screening methodology via polymerase chain reaction (PCR) was validated to (i) detect 5′ homologous recombination events; (ii) distinguish the wild-type, recombined, neo-excised, and Cre-excised alleles; and (iii) establish mouse genotypes (Figure 1B). After PCR identification of three ES cell clones with integration of the neomycin cassette in a heterozygous state and full sequencing into the surrounding locus for confirmation of genomic integrity, blastocyst injection generated three chimeric males with a chimerism rate above 50%. Three heterozygous floxed and (after crossbreeding with pan-Cre-deleter mice) three heterozygous constitutive mice were derived, with a second PCR screening performed to verify neo- and Cre-mediated excision events, followed by additional sequencing of the genomic locus. This approach generated 14 heterozygous floxed animals (7 males and 7 females) and 5 heterozygous constitutive KO mice (2 males, 3 females) in the F1 generation, which were interbred to generate F2 generations of the floxed conditional KO (Atxn2l-cKO) strain and the constitutive KO (Atxn2l-KO) strain of heterozygous breeders.

3.2. Crossbreeding with Constitutive Cre-Deleters Confirms Embryonic Lethality of Homozygous ATXN2L-Null Mice

Crossbreeding between heterozygous constitutive KO animals was performed to assess if the Atxn2l exon 10–17 deletion event causes embryonic lethality, similar to previously reported [83] constitutive Atxn2l exon 5–8 deletion, where the Lsm domain is missing (in addition to the absence of LsmAD/PAM2/Pat1 homology sequences in the current exon 10–17 strain). Among >100 collected offspring genotypes, no postnatal ATXN2L-null homozygote was observed (Table 1), in good agreement with the notion that embryonic lethality occurred again, despite the difference in targeted exons.

3.3. Crossbreeding with CamK2a-Dependent Cre/ERT2 Mice and Subsequent Tamoxifen Injection Generate Atxn2l-cKO in Adult Frontal Cortex Tissue

To selectively delete Atxn2l in CamK2a-positive neurons postnatally at the early adult age, homozygous Atxn2l-flox mice were obtained that differed regarding the heterozygous presence or absence of transgenic CamK2a-Cre/ERT2. Both were intraperitoneally administered tamoxifen over five consecutive days at ages of 2–3 months (Figure 2A). Their locomotor behavior was documented regularly until the age of 9 months, before tissues were dissected for further analyses (Figure 2B). PCR analyses at the DNA level in ear punches (Figure 2C) and at the RNA level in the frontal cortex (Figure 2D) confirmed the desired flox/Cre genotypes and demonstrated the successful Atxn2l deletion.

3.4. Atxn2l-cKO in Frontal Cortex Tissue Showed Mosaic Expression in CamK2a-Positive Neurons

To obtain a first impression of the cellular pattern of ATXN2L loss in the frontal cortex, immunofluorescence labeling for ATXN2L and CamK2a was employed. Serial brain sections of two cKO and two floxed WT mice were cut from the olfactory bulb to the hippocampus (one WT brain was discarded after postmortem genotyping). ATXN2L immunoreactivity was missing from many but not all CamK2a-positive neurons in the frontal cortex of the cKO mice (Figure 3) and hippocampus, demonstrating that either the transgenic CamK2a-Cre/ERT2 line or the tamoxifen dosage employed caused weak Cre expression, resulting in a mild chimeric deletion only in a part of the target cells. The observations in the brains investigated also indicate that ATXN2L deletion does not appear to cause widespread cell death or strong dedifferentiation of adult neurons even after >6 months.

3.5. CamK2a-Dependent Atxn2l-cKO Triggers Deficits in Spontaneous Horizontal Locomotion

To assess whether the absence of ATXN2L from the CamK2a+ neurons of the frontal cortex affects exploratory behavior, we quantified the spontaneous locomotor activity of mice after TAM injection in an open field paradigm after tamoxifen injection at monthly intervals from the ages of 3 to 9 months. The two weeks immediately after drug administration were exempted because animal handling with repeated intraperitoneal injections of tamoxifen dissolved in oil can transiently trigger discomfort or even peritonitis, resulting in a significant variability in behavior. The average spontaneous mobility parameters for cKO usually showed similar or lower values than floxed WT mice (except rest and stereotypy time), with consistent significant decreases for the parameter ambulatory time at 8 and 9 months (Figure 4). Overall, the data indicate that the chimeric dose reduction of ATXN2L in the CamK2a+ neurons of the frontal cortex was sufficient to alter curiosity and/or anxiety levels.

3.6. CamK2a-Dependent Atxn2l-cKO Mouse Frontal Cortex Proteomics Shows ATXN2L Protein Reduction to 75% and Dysregulation of the Alternative Splicing Pathway

To demonstrate the molecular consequences of ATXN2L-cKO in adult nervous tissue, samples from several important brain regions (olfactory bulb, frontal cortex, striatum, hippocampus, septum, tectum, and cerebellum) were analyzed using label-free mass spectrometry to quantify their global proteome profiles. In the frontal cortex, average ATXN2L protein abundance decreased to 75% in the four samples with nominal significance, after the tamoxifen-activated, Cre-mediated deletion events in CamK2a-positive neurons at ages >9 months (Figure 5, Table S1). This quantification result is credible, given that ATXN2L is physiologically present in these neurons, as well as in other neurons and glia, endothelial, and blood cells, where no deletion is expected in our experiment. The two proteins with significant ATXN2L dependence on murine embryonic fibroblasts—NUFIP2 as an RNA processing factor and SYNE2 as a bridge between the nuclear envelope and microtubules—did not display dysregulated levels (Table S1). In our complete analysis of four cKO samples, the strongest downregulation was observed for MAF1 as a repressor of RNA polymerases and the U6 snRNP, as well as the ribosomal translation apparatus, which is controlled by mTOR growth signaling [88]. Even more significant downregulation was observed for ALDH3B1 as a factor that protects medium-/long-chain fatty acids from lipid peroxidation. The strongest upregulation was documented for REEP3 as a bridge between the endoplasmic reticulum, with microtubules that ensure the nuclear envelope’s architecture [89,90].
Considering this mild decrease in ATXN2L levels upon CamK2a-dependent deletion, the downstream consequences would be too subtle for immunoblot analyses, and thus, only systematic bioinformatics surveys with alternate approaches were conducted.
STRING interaction and enrichment analysis revealed that protein dysregulations occurred with the strongest enrichment in dendrites (false discovery rate, FDR = 4.07 × 10−8); for cytoskeleton binding proteins (FDR = 4.36 × 10−5); and factors with rapid regulation by phosphorylation (FDR = 2.50 × 10−7), acetylation (FDR = 1.05 × 10−5), and alternative splicing (FDR = 9.61 × 10−5). The only enriched protein motifs were the pleckstrin homology domains (FDR = 0.04), which mediate binding to inositol lipids. As a single ATXN2L interactor with significantly dysregulated levels, NAA38 was reduced to 74% with nominal significance. NAA38 is a member of the snRNP family of Lsm domain-containing proteins and serves as an auxiliary component of the N-terminal acetyltransferase C (NatC) complex, which acts after ribosomal translation in the cytosol.
Other dysregulated RNA processing proteins with nominal significance included nuclear splicing factor SRSF11, RNA cytosine C(5)-methyltransferase NSUN2, and RPS3 and MRPL14 as ribosomal subunits in the cytosol and mitochondria, respectively; this was found in both the complete analysis of four cKO versus four floxed WT samples and in the enrichment analysis of three selected cKO mice with the lowest ATXN2L levels versus three floxed WT mice with the highest levels.
Upon assessing consistencies between the frontal cortex and hippocampal proteome profiles; normalization either among multiple brain regions; or normalization among these two regions with maximal ATXN2L depletion, an abundance of cytoplasmic ribonucleoprotein granule factors with nominal-significance dysregulations stood out (FDR = 0.0125). This involved decreases in ATXN2L and AGO3 versus increases in LSM3, EDC4, FXR2, NSUN2, LARP7, and SRSF11.
Overall, the mild CamK2a-dependent Atxn2l-cKO in the frontal cortex provided preliminary insights into the alterations in neural ribonucleoproteins and pathways that underlie the phenotypic deficits of spontaneous locomotion.

4. Discussion

Mutations of the less-abundant ATXN2 and the more-abundant ATXN2L have a preferential impact on neural tissues, with their distorted functions making causal contributions to the adult neurodegenerative diseases SCA2 and ALS. However, no mammalian model has been available where ATXN2L mutation effects can be studied in adult neurons. Furthermore, the primary protein–RNA interactions of ATXN2L in adult mammalian neurons have not been documented. Moreover, the exact physiological role of ATXN2L in RNA processing remains to be identified, both during growth periods, when its subcellular distribution shows perinuclear concentration, and in periods of cell damage, when its redistribution to stress granules suggests its involvement in quality control and repair.
Here, we generated the first Atxn2l-cKO mouse line via genetic ablation of exons 10–17 with a subsequent frameshift, interrupting ATXN2L N-terminal translation before the LsmAD and PAM2 domains and the C-terminal Pat1-homology region. Upon constitutive Cre-mediated deletion in homozygosity, embryonic lethality ensued, as previously reported for Atxn2l exon 5–8 deletion with a frameshift [83]. Upon conditional CamK2a-Cre/ERT2-mediated deletion in frontal cortex neurons via tamoxifen injection at the adult ages of 2–3 months, as well as subsequent aging to 9–12 months, cell death was not observed in CamK2a-positive neurons with completely absent ATXN2L. However, altered curiosity and/or anxiety were observed in response to the altered signaling of these neurons upon ATXN2L absence. Analyses of the global proteome of the frontal cortex (and hippocampus) from the Atxn2l-cKO mice confirmed a reduction in ATXN2L protein to 75% abundance, as well as weak downstream alterations in the alternative splicing pathway (e.g., SRSF11 and LARP7) and the cytoplasmic ribonucleoprotein granule composition. The ATXN2L protein is mainly cytoplasmic, and it appears to control the surveillance and triage of alternatively spliced isoforms, which need rapid turnover because of stress and stimulus. Our findings on the effects of ATXN2L Lsm and LsmAD are in excellent agreement with the well-established function of nuclear Sm domains for alternative splicing [91] and cytosolic Lsm1-7 rings for balancing mRNA translation versus turnover [92]. The rapid changes that occur between different alternative isoforms of any factor enable growth and compensate for stress; this ability appeared with the evolution of eukaryotic organisms [93], and indeed, Ataxin-2 family members also evolved in primitive eukaryotes. These organisms suffer from oxidative stress due to the endosymbiosis of mitochondria and chloroplasts. Failures in protective responses to radical oxygen species are a central cause of neurodegenerative processes, and physiological and pharmacological mechanisms of defense are being intensely explored, e.g., selenoproteins in the nervous system and the application of nano-selenium in treating mitochondrial problems [94,95].
Our observation of chimeric and mosaic deletions upon CamK2a-driven Cre/ERT2 expression and tamoxifen administration has been reported previously [96,97,98,99]. Similarly, altered curiosity-driven exploration and/or anxiety is an expected feature upon frontal cortex dysfunction [100,101,102]. Furthermore, an impact on alternative splicing was previously shown for mutations in TDP-43, FMR1, NUFIP2, and G3BP2 [103,104,105,106], as they are ATXN2/ATXN2L ribonucleoprotein interactors and stress granule components [82]. Thus, the results for the new Atxn2l-cKO mouse align with previous work.
The main limitations of this study derive from the choice of the CamK2a promoter to selectively drive weak Cre expression in the frontal cortex and hippocampus. Given that Cre transgene expression is weak when controlled by the CamK2a promoter, ATXN2L depletion was mild in the current project, and the downstream proteome dysregulations were too subtle for validation using independent techniques such as immunoblots and quantitative RT-qPCR. Therefore, to maximize the effect sizes of downstream proteome dysregulations, the next round of Atxn2l-cKO experiments could be driven by a strong promoter with specificity for forebrain and hippocampus projection neurons, such as the NEX-Cre transgene [107]. While affecting the frontal cortex and hippocampus is unlikely to restrict the survival of mouse mutants—thus providing a safe opportunity to assess the viability of ATXN2L depletion in adult neurons—future experiments should also target motor neurons, cerebellar neurons, and brainstem neurons, which are more critical and correspond to the neural circuits affected by ALS and SCA2. All current mass spectrometry findings must be regarded as preliminary, given that no single result achieved actual significance, and the findings varied in dependence on tamoxifen efficacy in different animals, diverse brain regions, and normalization approaches. However, it was illustrative to identify both NAA38 and LSM3 among the nominally significant dysregulations, given that ATXN2L and both factors mentioned are members of the Lsm protein family and that LSM12 was previously reported as an ATXN2L interactor [82]. The mainly nuclear ribonucleoproteins NSUN2 and SRSF11 were also consistently dysregulated, indicating that ATXN2L depletion leads to adaptations in nuclear RNA processing. NSUN2 acts with ALYREF and the ATXN2 interactor YBX1 to bind m5C-mRNAs and modify their nuclear export [108,109]. SRSF11 (also known as p54 or SRp54) always resides in the spliceosome [110,111], acting as a constitutive splicing factor, but it associates with U2AF65, unlike other members of the SR family [112]; furthermore, its specific functions include the splicing of small introns [113] and neuronal microexons [114].
Overall, this project generated the first mammalian conditional Atxn2l deletion strain, providing a proof of concept demonstrating that it constitutes a useful tool for future analyses of ATXN2L physiological functions in adult brains, which have selective importance for neuronal responses to stress and stimuli.

5. Conclusions

This study generated the first mouse strain with conditional deletion of ATXN2L, providing evidence that (i) the complete absence of ATXN2L is incompatible with embryonic development and (ii) the chimeric removal of ATXN2L protein levels from half of the CamK2a-positive frontal cortex neurons triggers reduced spontaneous locomotion and dysregulated protein levels in the alternative splicing pathway in adult mice.

Supplementary Materials

The following supporting information can be downloaded from https://www.mdpi.com/article/10.3390/cells14191532/s1, Table S1. Primers used for genotyping; Table S2. Proteome frontal cortex; Table S3. STRING analysis from proteome frontal cortex.

Author Contributions

Conceptualization, J.K. and G.A.; methodology, J.K., L.-E.A.-M., A.R.K., M.F., S.G., G.K., D.M. and T.D.; validation, L.-E.A.-M. and A.R.K.; formal analysis, J.K., L.-E.A.-M., D.M. and G.A.; investigation, J.K., L.-E.A.-M., S.G., D.M., M.F. and G.A.; resources, D.M., T.D. and G.A.; data curation, J.K., D.M. and G.A.; writing—original draft preparation, J.K., L.-E.A.-M. and G.A.; writing—review and editing, J.K., L.-E.A.-M., A.R.K., M.F., D.M., T.D. and G.A.; visualization, J.K., L.-E.A.-M., A.R.K., M.F., D.M. and G.A.; supervision, S.G., D.M. and G.A.; project administration, G.A.; funding acquisition, D.M. and G.A. All authors have read and agreed to the published version of the manuscript.

Funding

This study was funded by the Deutsche Forschungsgemeinschaft (DFG AU96/21-1).

Institutional Review Board Statement

The animal study protocol was approved by the Regierungspräsidium Darmstadt (V54-19c20/15-FK/2032, on 11 March 2019).

Data Availability Statement

All proteome data were deposited in PRIDE with accession number PXD064497.

Acknowledgments

Invaluable advice and support from Ann-Carol Eberle, Delphine Cartier, Patricia Isnard-Petit, and Kader Thiam at Genoway (Lyon, France) in the generation of conditional ATXN2L-null mice made this project possible. We thank Beata Lukaszewska-McGreal for proteome sample preparation and the Max Planck Society for support, as well as the ZFE staff at Goethe University Frankfurt Medical School for their animal care.

Conflicts of Interest

Thomas Deller received honoraria from Novartis for lectures on human brain anatomy. All other authors declare that this research was conducted in the absence of any commercial or financial relationships that could be construed as potential conflicts of interest.

Abbreviations

The following abbreviations are used in this manuscript:
AGO3Argonaute RISC Catalytic Component 3
ALDH3B1Medium-Chain Fatty Aldehyde Dehydrogenase
ALSAmyotrophic Lateral Sclerosis
ALYREFAly/REF Export Factor
ATGAutophagy-Related Gene
ATXAtaxin
ATXN2Ataxin-2
ATXN2LAtaxin-2-Like
AU-richAdenosin-Uridine Rich
BCABicinchoninic Acid
bpBase Pair
CAGCytosine–Adenine–Guanine Trinucleotide Repeat
CamK2aCalcium/Calmodulin-Dependent Protein Kinase II Alpha
cKOConditional Knock-Out
CreCyclization Recombination Enzyme
DEADAsp-Glu-Ala-Asp (DEAD-box helicase family)
DIAData-Independent Acquisition
DNADeoxyribo-Nucleic Acid
DTADiphtheria Toxin Fragment A
DxxDAspartate–Any Amino Acid–Any Amino Acid–Aspartate
EDC4Enhancer of mRNA Decapping 4
EGFEpidermal Growth Factor
EREndoplasmic Reticulum
ERT2Tamoxifen-Inducible Estrogen Receptor Domain, Improved Version
ESEmbryonic Stem Cell
FDRFalse Discovery Rate
FEBSFederation of European Biochemical Societies
FIJIFIJI Is Just ImageJ
FloxedSequence Flanked by Two loxP Sites
FMRPFragile X Mental Retardation Protein
FMR1Fragile X Messenger Ribonucleoprotein 1
FXR2Fragile X Mental Retardation, Autosomal Homolog 2
GOGene Ontology
G3BP2GTPase Activating Protein (SH3 Domain) Binding Protein 2
hATXN2Human Ataxin-2
hetHeterozygous
homHomozygous
HSCHematopoietic Stem Cell
kbKilo-Base
KEGGKyoto Encyclopedia of Genes and Genomes
KOKnock-Out
LARP7La Ribonucleoprotein 7, Transcription Regulator, Binds U6 snRNA
LCLiquid Chromatography
LEDLight Emitting Diode
LoxPLocus of X-Over (Crossing-Over) in Bacteriophage P1
LsmLike-Sm Domain
LsmADLike-Sm-Associated Domain
LSM3LSM3 Homolog, U6 Small Nuclear RNA-Associated
MAF1MAF1 Homolog, Negative Regulator of RNA Polymerase III
MPLMyelo-Proliferative Leukaemia Protein
mRNAMessenger Ribo-Nucleic Acid
MRPL14Large Ribosomal Subunit Protein UL14m
MSMass Spectrometry
mTORMechanistic Target of Rapamycin
mTORC1Mechanistic Target of Rapamycin-Complex-Associated Protein 1
m5C5-methyl-Cytosine
NAA38N-Alpha-Acetyltransferase 38, NatC Auxiliary Subunit
NGSNormal Goat Serum
NSUN2NOP2/Sun RNA Methyltransferase 2
NUFIP2Nuclear Fragile X Mental Retardation Protein Interacting Protein 2
oligo(U)Several (Uridine Bases)
OROdds Ratio
PABPPoly(A)-Binding Protein
PAM2Poly(A)-Binding protein association Motif type 2
PASEFParallel Accumulation Serial Fragmentation
Pat1Yeast Factor for Protection of mRNA 3′-UTRs from Trimming
P-bodiesProcessing Bodies in the Cytosol, Where RNA Is Degraded
Pbp1Poly(A)-Binding Protein 1 in Yeast
PBSPhosphate-Buffered Saline
PCRPolymerase Chain Reaction
Poly(A)many (Adenine bases)
polyQMany Glutamine Amino Acids
PRMProline-Rich Motif
REEP3Receptor Expression-Enhancing Protein 3
RNARibo-Nucleic Acid
RNPRibo-Nucleoprotein
RoxPloxP-Analogous Site, Recognized by Phage Integrase Dre
RPS3Small Ribosomal Subunit Protein US3
RRMRNA Recognition Motif
rRNARibosomal Ribo-Nucleic Acid
RTReverse Transcription
SCA2Spinocerebellar Ataxia type 2
SDStandard Deviation
SEMStandard Error of the Mean
SGStress Granule
siRNASmall Interfering RNA
SNSubstantia Nigra
SNPSingle Nucleotide Polymorphism
snRNASmall Nuclear Ribo-Nucleic Acid
snRNPSmall Nuclear Ribo-Nucleic-Acid Binding Protein
SRSerine/Arginine-Rich Protein, Family of Splicing Factors
SRSF11Serine and Arginine Rich Splicing Factor 11
SYNE2Spectrin Repeat Containing Nuclear Envelope Protein 2
TAMTamoxifen
TDP-43TAR DNA-Binding Protein-43
TgTransgenic
tRNATransfer Ribo-Nucleic Acid
UPRUnfolded Protein Response
UTRUntranslated Region of mRNA
U2AF65U2 Small Nuclear RNA Auxiliary Factor 2
WBWestern Blot
WTWild-Type
YBX1Y-Box-Binding Protein 1, CCAAT-Binding Transcription Factor I
ZFEZentrale Forschungseinrichtung (Central Animal Facility)

References

  1. Achsel, T.; Stark, H.; Luhrmann, R. The Sm domain is an ancient RNA-binding motif with oligo(U) specificity. Proc. Natl. Acad. Sci. USA 2001, 98, 3685–3689. [Google Scholar] [CrossRef]
  2. Tharun, S.; He, W.; Mayes, A.E.; Lennertz, P.; Beggs, J.D.; Parker, R. Yeast Sm-like proteins function in mRNA decapping and decay. Nature 2000, 404, 515–518. [Google Scholar] [CrossRef]
  3. Mura, C.; Randolph, P.S.; Patterson, J.; Cozen, A.E. Archaeal and eukaryotic homologs of Hfq: A structural and evolutionary perspective on Sm function. RNA Biol. 2013, 10, 636–651. [Google Scholar] [CrossRef]
  4. Swisher, K.D.; Parker, R. Localization to, and effects of Pbp1, Pbp4, Lsm12, Dhh1, and Pab1 on stress granules in Saccharomyces cerevisiae. PLoS ONE 2010, 5, e10006. [Google Scholar] [CrossRef] [PubMed]
  5. Seidel, G.; Meierhofer, D.; Sen, N.E.; Guenther, A.; Krobitsch, S.; Auburger, G. Quantitative Global Proteomics of Yeast PBP1 Deletion Mutants and Their Stress Responses Identifies Glucose Metabolism, Mitochondrial, and Stress Granule Changes. J. Proteome Res. 2017, 16, 504–515. [Google Scholar] [CrossRef]
  6. Yang, Y.S.; Kato, M.; Wu, X.; Litsios, A.; Sutter, B.M.; Wang, Y.; Hsu, C.H.; Wood, N.E.; Lemoff, A.; Mirzaei, H.; et al. Yeast Ataxin-2 Forms an Intracellular Condensate Required for the Inhibition of TORC1 Signaling during Respiratory Growth. Cell 2019, 177, 697–710.E17. [Google Scholar] [CrossRef]
  7. Kato, M.; Yang, Y.S.; Sutter, B.M.; Wang, Y.; McKnight, S.L.; Tu, B.P. Redox State Controls Phase Separation of the Yeast Ataxin-2 Protein via Reversible Oxidation of Its Methionine-Rich Low-Complexity Domain. Cell 2019, 177, 711–721.E8. [Google Scholar] [CrossRef]
  8. Kiehl, T.R.; Shibata, H.; Pulst, S.M. The ortholog of human ataxin-2 is essential for early embryonic patterning in C. elegans. J. Mol. Neurosci. 2000, 15, 231–241. [Google Scholar] [CrossRef] [PubMed]
  9. Ciosk, R.; DePalma, M.; Priess, J.R. ATX-2, the C. elegans ortholog of ataxin 2, functions in translational regulation in the germline. Development 2004, 131, 4831–4841. [Google Scholar] [CrossRef]
  10. Bar, D.Z.; Charar, C.; Dorfman, J.; Yadid, T.; Tafforeau, L.; Lafontaine, D.L.; Gruenbaum, Y. Cell size and fat content of dietary-restricted Caenorhabditis elegans are regulated by ATX-2, an mTOR repressor. Proc. Natl. Acad. Sci. USA 2016, 113, E4620–E4629. [Google Scholar] [CrossRef] [PubMed]
  11. Stubenvoll, M.D.; Medley, J.C.; Irwin, M.; Song, M.H. ATX-2, the C. elegans Ortholog of Human Ataxin-2, Regulates Centrosome Size and Microtubule Dynamics. PLoS Genet. 2016, 12, e1006370. [Google Scholar] [CrossRef]
  12. Del Castillo, U.; Gnazzo, M.M.; Sorensen Turpin, C.G.; Nguyen, K.C.Q.; Semaya, E.; Lam, Y.; de Cruz, M.A.; Bembenek, J.N.; Hall, D.H.; Riggs, B.; et al. Conserved role for Ataxin-2 in mediating endoplasmic reticulum dynamics. Traffic 2019, 20, 436–447. [Google Scholar] [CrossRef]
  13. Beath, E.A.; Bailey, C.; Mahantesh Magadam, M.; Qiu, S.; McNally, K.L.; McNally, F.J. Katanin, kinesin-13, and ataxin-2 inhibit premature interaction between maternal and paternal genomes in C. elegans zygotes. Elife 2024, 13, RP97812. [Google Scholar] [CrossRef]
  14. Satterfield, T.F.; Jackson, S.M.; Pallanck, L.J. A Drosophila homolog of the polyglutamine disease gene SCA2 is a dosage-sensitive regulator of actin filament formation. Genetics 2002, 162, 1687–1702. [Google Scholar] [CrossRef] [PubMed]
  15. Satterfield, T.F.; Pallanck, L.J. Ataxin-2 and its Drosophila homolog, ATX2, physically assemble with polyribosomes. Hum. Mol. Genet. 2006, 15, 2523–2532. [Google Scholar] [CrossRef]
  16. Al-Ramahi, I.; Perez, A.M.; Lim, J.; Zhang, M.; Sorensen, R.; de Haro, M.; Branco, J.; Pulst, S.M.; Zoghbi, H.Y.; Botas, J. dAtaxin-2 mediates expanded Ataxin-1-induced neurodegeneration in a Drosophila model of SCA1. PLoS Genet. 2007, 3, e234. [Google Scholar] [CrossRef]
  17. McCann, C.; Holohan, E.E.; Das, S.; Dervan, A.; Larkin, A.; Lee, J.A.; Rodrigues, V.; Parker, R.; Ramaswami, M. The Ataxin-2 protein is required for microRNA function and synapse-specific long-term olfactory habituation. Proc. Natl. Acad. Sci. USA 2011, 108, E655–E662. [Google Scholar] [CrossRef] [PubMed]
  18. Lim, C.; Allada, R. ATAXIN-2 activates PERIOD translation to sustain circadian rhythms in Drosophila. Science 2013, 340, 875–879. [Google Scholar] [CrossRef] [PubMed]
  19. Zhang, Y.; Ling, J.; Yuan, C.; Dubruille, R.; Emery, P. A role for Drosophila ATX2 in activation of PER translation and circadian behavior. Science 2013, 340, 879–882. [Google Scholar] [CrossRef]
  20. Sudhakaran, I.P.; Hillebrand, J.; Dervan, A.; Das, S.; Holohan, E.E.; Hulsmeier, J.; Sarov, M.; Parker, R.; VijayRaghavan, K.; Ramaswami, M. FMRP and Ataxin-2 function together in long-term olfactory habituation and neuronal translational control. Proc. Natl. Acad. Sci. USA 2014, 111, E99–E108. [Google Scholar] [CrossRef]
  21. Vianna, M.C.; Poleto, D.C.; Gomes, P.F.; Valente, V.; Paco-Larson, M.L. Drosophila ataxin-2 gene encodes two differentially expressed isoforms and its function in larval fat body is crucial for development of peripheral tissues. FEBS Open Bio 2016, 6, 1040–1053. [Google Scholar] [CrossRef]
  22. Lee, J.; Yoo, E.; Lee, H.; Park, K.; Hur, J.H.; Lim, C. LSM12 and ME31B/DDX6 Define Distinct Modes of Posttranscriptional Regulation by ATAXIN-2 Protein Complex in Drosophila Circadian Pacemaker Neurons. Mol. Cell 2017, 66, 129–140.e7. [Google Scholar] [CrossRef] [PubMed]
  23. Bakthavachalu, B.; Huelsmeier, J.; Sudhakaran, I.P.; Hillebrand, J.; Singh, A.; Petrauskas, A.; Thiagarajan, D.; Sankaranarayanan, M.; Mizoue, L.; Anderson, E.N.; et al. RNP-Granule Assembly via Ataxin-2 Disordered Domains Is Required for Long-Term Memory and Neurodegeneration. Neuron 2018, 98, 754–766. [Google Scholar] [CrossRef]
  24. Cha, I.J.; Lee, D.; Park, S.S.; Chung, C.G.; Kim, S.Y.; Jo, M.G.; Kim, S.Y.; Lee, B.H.; Lee, Y.S.; Lee, S.B. Ataxin-2 Dysregulation Triggers a Compensatory Fragile X Mental Retardation Protein Decrease in Drosophila C4da Neurons. Mol. Cells 2020, 43, 870–879. [Google Scholar] [CrossRef]
  25. Singh, A.; Hulsmeier, J.; Kandi, A.R.; Pothapragada, S.S.; Hillebrand, J.; Petrauskas, A.; Agrawal, K.; Rt, K.; Thiagarajan, D.; Jayaprakashappa, D.; et al. Antagonistic roles for Ataxin-2 structured and disordered domains in RNP condensation. Elife 2021, 10, e60326. [Google Scholar] [CrossRef]
  26. Del Castillo, U.; Norkett, R.; Lu, W.; Serpinskaya, A.; Gelfand, V.I. Ataxin-2 is essential for cytoskeletal dynamics and neurodevelopment in Drosophila. iScience 2022, 25, 103536. [Google Scholar] [CrossRef]
  27. Corgiat, E.B.; List, S.M.; Rounds, J.C.; Yu, D.; Chen, P.; Corbett, A.H.; Moberg, K.H. The Nab2 RNA-binding protein patterns dendritic and axonal projections through a planar cell polarity-sensitive mechanism. G3 2022, 12, jkac100. [Google Scholar] [CrossRef] [PubMed]
  28. Petrauskas, A.; Fortunati, D.L.; Kandi, A.R.; Pothapragada, S.S.; Agrawal, K.; Singh, A.; Huelsmeier, J.; Hillebrand, J.; Brown, G.; Chaturvedi, D.; et al. Structured and disordered regions of Ataxin-2 contribute differently to the specificity and efficiency of mRNP granule formation. PLoS Genet. 2024, 20, e1011251. [Google Scholar] [CrossRef] [PubMed]
  29. Auburger, G.; Sen, N.E.; Meierhofer, D.; Basak, A.N.; Gitler, A.D. Efficient Prevention of Neurodegenerative Diseases by Depletion of Starvation Response Factor Ataxin-2. Trends Neurosci. 2017, 40, 507–516. [Google Scholar] [CrossRef]
  30. Jimenez-Lopez, D.; Guzman, P. Insights into the evolution and domain structure of Ataxin-2 proteins across eukaryotes. BMC Res. Notes 2014, 7, 453. [Google Scholar] [CrossRef]
  31. Pulst, S.M.; Nechiporuk, A.; Nechiporuk, T.; Gispert, S.; Chen, X.N.; Lopes-Cendes, I.; Pearlman, S.; Starkman, S.; Orozco-Diaz, G.; Lunkes, A.; et al. Moderate expansion of a normally biallelic trinucleotide repeat in spinocerebellar ataxia type 2. Nat. Genet. 1996, 14, 269–276. [Google Scholar] [CrossRef]
  32. Sanpei, K.; Takano, H.; Igarashi, S.; Sato, T.; Oyake, M.; Sasaki, H.; Wakisaka, A.; Tashiro, K.; Ishida, Y.; Ikeuchi, T.; et al. Identification of the spinocerebellar ataxia type 2 gene using a direct identification of repeat expansion and cloning technique, DIRECT. Nat. Genet. 1996, 14, 277–284. [Google Scholar] [CrossRef]
  33. Imbert, G.; Saudou, F.; Yvert, G.; Devys, D.; Trottier, Y.; Garnier, J.M.; Weber, C.; Mandel, J.L.; Cancel, G.; Abbas, N.; et al. Cloning of the gene for spinocerebellar ataxia 2 reveals a locus with high sensitivity to expanded CAG/glutamine repeats. Nat. Genet. 1996, 14, 285–291. [Google Scholar] [CrossRef]
  34. Velazquez-Perez, L.; Seifried, C.; Santos-Falcon, N.; Abele, M.; Ziemann, U.; Almaguer, L.E.; Martinez-Gongora, E.; Sanchez-Cruz, G.; Canales, N.; Perez-Gonzalez, R.; et al. Saccade velocity is controlled by polyglutamine size in spinocerebellar ataxia 2. Ann. Neurol. 2004, 56, 444–447. [Google Scholar] [CrossRef]
  35. Rub, U.; Gierga, K.; Brunt, E.R.; de Vos, R.A.; Bauer, M.; Schols, L.; Burk, K.; Auburger, G.; Bohl, J.; Schultz, C.; et al. Spinocerebellar ataxias types 2 and 3: Degeneration of the pre-cerebellar nuclei isolates the three phylogenetically defined regions of the cerebellum. J. Neural Transm. 2005, 112, 1523–1545. [Google Scholar] [CrossRef] [PubMed]
  36. Gierga, K.; Burk, K.; Bauer, M.; Orozco Diaz, G.; Auburger, G.; Schultz, C.; Vuksic, M.; Schols, L.; de Vos, R.A.; Braak, H.; et al. Involvement of the cranial nerves and their nuclei in spinocerebellar ataxia type 2 (SCA2). Acta Neuropathol. 2005, 109, 617–631. [Google Scholar] [CrossRef] [PubMed]
  37. Ralser, M.; Nonhoff, U.; Albrecht, M.; Lengauer, T.; Wanker, E.E.; Lehrach, H.; Krobitsch, S. Ataxin-2 and huntingtin interact with endophilin-A complexes to function in plastin-associated pathways. Hum. Mol. Genet. 2005, 14, 2893–2909. [Google Scholar] [CrossRef]
  38. Tuin, I.; Voss, U.; Kang, J.S.; Kessler, K.; Rub, U.; Nolte, D.; Lochmuller, H.; Tinschert, S.; Claus, D.; Krakow, K.; et al. Stages of sleep pathology in spinocerebellar ataxia type 2 (SCA2). Neurology 2006, 67, 1966–1972. [Google Scholar] [CrossRef] [PubMed]
  39. Lastres-Becker, I.; Brodesser, S.; Lutjohann, D.; Azizov, M.; Buchmann, J.; Hintermann, E.; Sandhoff, K.; Schurmann, A.; Nowock, J.; Auburger, G. Insulin receptor and lipid metabolism pathology in ataxin-2 knock-out mice. Hum. Mol. Genet. 2008, 17, 1465–1481. [Google Scholar] [CrossRef]
  40. Lastres-Becker, I.; Rub, U.; Auburger, G. Spinocerebellar ataxia 2 (SCA2). Cerebellum 2008, 7, 115–124. [Google Scholar] [CrossRef]
  41. Nonis, D.; Schmidt, M.H.H.; van de Loo, S.; Eich, F.; Dikic, I.; Nowock, J.; Auburger, G. Ataxin-2 associates with the endocytosis complex and affects EGF receptor trafficking. Cell. Signal 2008, 20, 1725–1739. [Google Scholar] [CrossRef] [PubMed]
  42. Rub, U.; Del Turco, D.; Del Tredici, K.; de Vos, R.A.; Brunt, E.R.; Reifenberger, G.; Seifried, C.; Schultz, C.; Auburger, G.; Braak, H. Thalamic involvement in a spinocerebellar ataxia type 2 (SCA2) and a spinocerebellar ataxia type 3 (SCA3) patient, and its clinical relevance. Brain 2003, 126, 2257–2272. [Google Scholar] [CrossRef]
  43. van de Loo, S.; Eich, F.; Nonis, D.; Auburger, G.; Nowock, J. Ataxin-2 associates with rough endoplasmic reticulum. Exp. Neurol. 2009, 215, 110–118. [Google Scholar] [CrossRef]
  44. Almaguer-Mederos, L.E.; Falcon, N.S.; Almira, Y.R.; Zaldivar, Y.G.; Almarales, D.C.; Gongora, E.M.; Herrera, M.P.; Batallan, K.E.; Arminan, R.R.; Manresa, M.V.; et al. Estimation of the age at onset in spinocerebellar ataxia type 2 Cuban patients by survival analysis. Clin. Genet. 2010, 78, 169–174. [Google Scholar] [CrossRef]
  45. Auburger, G.W. Spinocerebellar ataxia type 2. Handb. Clin. Neurol. 2012, 103, 423–436. [Google Scholar] [CrossRef]
  46. Rub, U.; Schols, L.; Paulson, H.; Auburger, G.; Kermer, P.; Jen, J.C.; Seidel, K.; Korf, H.W.; Deller, T. Clinical features, neurogenetics and neuropathology of the polyglutamine spinocerebellar ataxias type 1, 2, 3, 6 and 7. Prog. Neurobiol. 2013, 104, 38–66. [Google Scholar] [CrossRef]
  47. Schols, L.; Reimold, M.; Seidel, K.; Globas, C.; Brockmann, K.; Hauser, T.K.; Auburger, G.; Burk, K.; den Dunnen, W.; Reischl, G.; et al. No parkinsonism in SCA2 and SCA3 despite severe neurodegeneration of the dopaminergic substantia nigra. Brain 2015, 138, 3316–3326. [Google Scholar] [CrossRef] [PubMed]
  48. Meierhofer, D.; Halbach, M.; Sen, N.E.; Gispert, S.; Auburger, G. Ataxin-2 (Atxn2)-Knock-Out Mice Show Branched Chain Amino Acids and Fatty Acids Pathway Alterations. Mol. Cell. Proteom. 2016, 15, 1728–1739. [Google Scholar] [CrossRef]
  49. Halbach, M.V.; Gispert, S.; Stehning, T.; Damrath, E.; Walter, M.; Auburger, G. Atxn2 Knockout and CAG42-Knock-in Cerebellum Shows Similarly Dysregulated Expression in Calcium Homeostasis Pathway. Cerebellum 2017, 16, 68–81. [Google Scholar] [CrossRef]
  50. Lastres-Becker, I.; Nonis, D.; Eich, F.; Klinkenberg, M.; Gorospe, M.; Kotter, P.; Klein, F.A.; Kedersha, N.; Auburger, G. Mammalian ataxin-2 modulates translation control at the pre-initiation complex via PI3K/mTOR and is induced by starvation. Biochim. Biophys. Acta 2016, 1862, 1558–1569. [Google Scholar] [CrossRef] [PubMed]
  51. Seidel, K.; Siswanto, S.; Fredrich, M.; Bouzrou, M.; den Dunnen, W.F.A.; Ozerden, I.; Korf, H.W.; Melegh, B.; de Vries, J.J.; Brunt, E.R.; et al. On the distribution of intranuclear and cytoplasmic aggregates in the brainstem of patients with spinocerebellar ataxia type 2 and 3. Brain Pathol. 2017, 27, 345–355. [Google Scholar] [CrossRef] [PubMed]
  52. Sen, N.E.; Canet-Pons, J.; Halbach, M.V.; Arsovic, A.; Pilatus, U.; Chae, W.H.; Kaya, Z.E.; Seidel, K.; Rollmann, E.; Mittelbronn, M.; et al. Generation of an Atxn2-CAG100 knock-in mouse reveals N-acetylaspartate production deficit due to early Nat8l dysregulation. Neurobiol. Dis. 2019, 132, 104559. [Google Scholar] [CrossRef]
  53. Xu, F.; Kula-Eversole, E.; Iwanaszko, M.; Lim, C.; Allada, R. Ataxin2 functions via CrebA to mediate Huntingtin toxicity in circadian clock neurons. PLoS Genet. 2019, 15, e1008356. [Google Scholar] [CrossRef]
  54. Elden, A.C.; Kim, H.J.; Hart, M.P.; Chen-Plotkin, A.S.; Johnson, B.S.; Fang, X.; Armakola, M.; Geser, F.; Greene, R.; Lu, M.M.; et al. Ataxin-2 intermediate-length polyglutamine expansions are associated with increased risk for ALS. Nature 2010, 466, 1069–1075. [Google Scholar] [CrossRef]
  55. Becker, L.A.; Huang, B.; Bieri, G.; Ma, R.; Knowles, D.A.; Jafar-Nejad, P.; Messing, J.; Kim, H.J.; Soriano, A.; Auburger, G.; et al. Therapeutic reduction of ataxin-2 extends lifespan and reduces pathology in TDP-43 mice. Nature 2017, 544, 367–371. [Google Scholar] [CrossRef]
  56. Gispert, S.; Kurz, A.; Waibel, S.; Bauer, P.; Liepelt, I.; Geisen, C.; Gitler, A.D.; Becker, T.; Weber, M.; Berg, D.; et al. The modulation of Amyotrophic Lateral Sclerosis risk by ataxin-2 intermediate polyglutamine expansions is a specific effect. Neurobiol. Dis. 2012, 45, 356–361. [Google Scholar] [CrossRef]
  57. Lahut, S.; Omur, O.; Uyan, O.; Agim, Z.S.; Ozoguz, A.; Parman, Y.; Deymeer, F.; Oflazer, P.; Koc, F.; Ozcelik, H.; et al. ATXN2 and its neighbouring gene SH2B3 are associated with increased ALS risk in the Turkish population. PLoS ONE 2012, 7, e42956. [Google Scholar] [CrossRef]
  58. Lee, T.; Li, Y.R.; Ingre, C.; Weber, M.; Grehl, T.; Gredal, O.; de Carvalho, M.; Meyer, T.; Tysnes, O.B.; Auburger, G.; et al. Ataxin-2 intermediate-length polyglutamine expansions in European ALS patients. Hum. Mol. Genet. 2011, 20, 1697–1700. [Google Scholar] [CrossRef] [PubMed]
  59. Ralser, M.; Albrecht, M.; Nonhoff, U.; Lengauer, T.; Lehrach, H.; Krobitsch, S. An integrative approach to gain insights into the cellular function of human ataxin-2. J. Mol. Biol. 2005, 346, 203–214. [Google Scholar] [CrossRef] [PubMed]
  60. Nonhoff, U.; Ralser, M.; Welzel, F.; Piccini, I.; Balzereit, D.; Yaspo, M.L.; Lehrach, H.; Krobitsch, S. Ataxin-2 interacts with the DEAD/H-box RNA helicase DDX6 and interferes with P-bodies and stress granules. Mol. Biol. Cell 2007, 18, 1385–1396. [Google Scholar] [CrossRef] [PubMed]
  61. Damrath, E.; Heck, M.V.; Gispert, S.; Azizov, M.; Nowock, J.; Seifried, C.; Rub, U.; Walter, M.; Auburger, G. ATXN2-CAG42 sequesters PABPC1 into insolubility and induces FBXW8 in cerebellum of old ataxic knock-in mice. PLoS Genet. 2012, 8, e1002920. [Google Scholar] [CrossRef]
  62. Kaehler, C.; Isensee, J.; Nonhoff, U.; Terrey, M.; Hucho, T.; Lehrach, H.; Krobitsch, S. Ataxin-2-like is a regulator of stress granules and processing bodies. PLoS ONE 2012, 7, e50134. [Google Scholar] [CrossRef]
  63. Yokoshi, M.; Li, Q.; Yamamoto, M.; Okada, H.; Suzuki, Y.; Kawahara, Y. Direct binding of Ataxin-2 to distinct elements in 3′ UTRs promotes mRNA stability and protein expression. Mol. Cell 2014, 55, 186–198. [Google Scholar] [CrossRef]
  64. Fittschen, M.; Lastres-Becker, I.; Halbach, M.V.; Damrath, E.; Gispert, S.; Azizov, M.; Walter, M.; Muller, S.; Auburger, G. Genetic ablation of ataxin-2 increases several global translation factors in their transcript abundance but decreases translation rate. Neurogenetics 2015, 16, 181–192. [Google Scholar] [CrossRef]
  65. Inagaki, H.; Hosoda, N.; Tsuiji, H.; Hoshino, S.I. Direct evidence that Ataxin-2 is a translational activator mediating cytoplasmic polyadenylation. J. Biol. Chem. 2020, 295, 15810–15825. [Google Scholar] [CrossRef]
  66. Canet-Pons, J.; Sen, N.E.; Arsovic, A.; Almaguer-Mederos, L.E.; Halbach, M.V.; Key, J.; Doring, C.; Kerksiek, A.; Picchiarelli, G.; Cassel, R.; et al. Atxn2-CAG100-KnockIn mouse spinal cord shows progressive TDP43 pathology associated with cholesterol biosynthesis suppression. Neurobiol. Dis. 2021, 152, 105289. [Google Scholar] [CrossRef] [PubMed]
  67. Boeynaems, S.; Dorone, Y.; Zhuang, Y.; Shabardina, V.; Huang, G.; Marian, A.; Kim, G.; Sanyal, A.; Sen, N.E.; Griffith, D.; et al. Poly(A)-binding protein is an ataxin-2 chaperone that regulates biomolecular condensates. Mol. Cell 2023, 83, 2020–2034.e6. [Google Scholar] [CrossRef] [PubMed]
  68. Zhuang, Y.; Li, Z.; Xiong, S.; Sun, C.; Li, B.; Wu, S.A.; Lyu, J.; Shi, X.; Yang, L.; Chen, Y.; et al. Circadian clocks are modulated by compartmentalized oscillating translation. Cell 2023, 186, 3245–3260.e23. [Google Scholar] [CrossRef]
  69. Wang, J.Y.; Liu, Y.J.; Zhang, X.L.; Liu, Y.H.; Jiang, L.L.; Hu, H.Y. PolyQ-expanded ataxin-2 aggregation impairs cellular processing-body homeostasis via sequestering the RNA helicase DDX6. J. Biol. Chem. 2024, 300, 107413. [Google Scholar] [CrossRef]
  70. Zhang, S.; Zhang, Y.; Chen, T.; Hu, H.Y.; Lu, C. The LSmAD Domain of Ataxin-2 Modulates the Structure and RNA Binding of Its Preceding LSm Domain. Cells 2025, 14, 383. [Google Scholar] [CrossRef] [PubMed]
  71. Drost, J.; Nonis, D.; Eich, F.; Leske, O.; Damrath, E.; Brunt, E.R.; Lastres-Becker, I.; Heumann, R.; Nowock, J.; Auburger, G. Ataxin-2 modulates the levels of Grb2 and SRC but not ras signaling. J. Mol. Neurosci. 2013, 51, 68–81. [Google Scholar] [CrossRef]
  72. Meunier, C.; Bordereaux, D.; Porteu, F.; Gisselbrecht, S.; Chretien, S.; Courtois, G. Cloning and characterization of a family of proteins associated with Mpl. J. Biol. Chem. 2002, 277, 9139–9147. [Google Scholar] [CrossRef] [PubMed]
  73. Coller, J.; Parker, R. General translational repression by activators of mRNA decapping. Cell 2005, 122, 875–886. [Google Scholar] [CrossRef]
  74. Lobel, J.H.; Gross, J.D. Pdc2/Pat1 increases the range of decay factors and RNA bound by the Lsm1-7 complex. RNA 2020, 26, 1380–1388. [Google Scholar] [CrossRef]
  75. Hurst, Z.; Liu, W.; Shi, Q.; Herman, P.K. A distinct P-body-like granule is induced in response to the disruption of microtubule integrity in Saccharomyces cerevisiae. Genetics 2022, 222, iyac105. [Google Scholar] [CrossRef]
  76. Vijjamarri, A.K.; Gupta, N.; Onu, C.; Niu, X.; Zhang, F.; Kumar, R.; Lin, Z.; Greenberg, M.L.; Hinnebusch, A.G. mRNA decapping activators Pat1 and Dhh1 regulate transcript abundance and translation to tune cellular responses to nutrient availability. Nucleic Acids Res. 2023, 51, 9314–9336. [Google Scholar] [CrossRef]
  77. Bahassou-Benamri, R.; Davin, A.H.; Gaillard, J.C.; Alonso, B.; Odorico, M.; Pible, O.; Armengaud, J.; Godon, C. Subcellular localization and interaction network of the mRNA decay activator Pat1 upon UV stress. Yeast 2013, 30, 353–363. [Google Scholar] [CrossRef]
  78. Vindry, C.; Marnef, A.; Broomhead, H.; Twyffels, L.; Ozgur, S.; Stoecklin, G.; Llorian, M.; Smith, C.W.; Mata, J.; Weil, D.; et al. Dual RNA Processing Roles of Pat1b via Cytoplasmic Lsm1-7 and Nuclear Lsm2-8 Complexes. Cell Rep. 2017, 20, 1187–1200. [Google Scholar] [CrossRef] [PubMed]
  79. Vindry, C.; Weil, D.; Standart, N. Pat1 RNA-binding proteins: Multitasking shuttling proteins. Wiley Interdiscip. Rev. RNA 2019, 10, e1557. [Google Scholar] [CrossRef] [PubMed]
  80. Pradhan, S.J.; Nesler, K.R.; Rosen, S.F.; Kato, Y.; Nakamura, A.; Ramaswami, M.; Barbee, S.A. The conserved P body component HPat/Pat1 negatively regulates synaptic terminal growth at the larval Drosophila neuromuscular junction. J. Cell Sci. 2012, 125, 6105–6116. [Google Scholar] [CrossRef]
  81. Kaehler, C.; Guenther, A.; Uhlich, A.; Krobitsch, S. PRMT1-mediated arginine methylation controls ATXN2L localization. Exp. Cell Res. 2015, 334, 114–125. [Google Scholar] [CrossRef] [PubMed]
  82. Key, J.; Almaguer-Mederos, L.E.; Kandi, A.R.; Sen, N.E.; Gispert, S.; Kopf, G.; Meierhofer, D.; Auburger, G. ATXN2L primarily interacts with NUFIP2, the absence of ATXN2L results in NUFIP2 depletion, and the ATXN2-polyQ expansion triggers NUFIP2 accumulation. Neurobiol. Dis. 2025, 209, 106903. [Google Scholar] [CrossRef]
  83. Key, J.; Harter, P.N.; Sen, N.E.; Gradhand, E.; Auburger, G.; Gispert, S. Mid-Gestation lethality of Atxn2l-Ablated Mice. Int. J. Mol. Sci. 2020, 21, 5124. [Google Scholar] [CrossRef] [PubMed]
  84. Truett, G.E.; Heeger, P.; Mynatt, R.L.; Truett, A.A.; Walker, J.A.; Warman, M.L. Preparation of PCR-quality mouse genomic DNA with hot sodium hydroxide and tris (HotSHOT). Biotechniques 2000, 29, 52–54. [Google Scholar] [CrossRef]
  85. Schindelin, J.; Arganda-Carreras, I.; Frise, E.; Kaynig, V.; Longair, M.; Pietzsch, T.; Preibisch, S.; Rueden, C.; Saalfeld, S.; Schmid, B.; et al. Fiji: An open-source platform for biological-image analysis. Nat. Methods 2012, 9, 676–682. [Google Scholar] [CrossRef]
  86. Martens, L.; Hermjakob, H.; Jones, P.; Adamski, M.; Taylor, C.; States, D.; Gevaert, K.; Vandekerckhove, J.; Apweiler, R. PRIDE: The proteomics identifications database. Proteomics 2005, 5, 3537–3545. [Google Scholar] [CrossRef]
  87. Szklarczyk, D.; Kirsch, R.; Koutrouli, M.; Nastou, K.; Mehryary, F.; Hachilif, R.; Gable, A.L.; Fang, T.; Doncheva, N.T.; Pyysalo, S.; et al. The STRING database in 2023: Protein-protein association networks and functional enrichment analyses for any sequenced genome of interest. Nucleic Acids Res. 2023, 51, D638–D646. [Google Scholar] [CrossRef] [PubMed]
  88. Zhang, S.; Li, X.; Wang, H.Y.; Steven Zheng, X.F. Beyond regulation of pol III: Role of MAF1 in growth, metabolism, aging and cancer. Biochim. Biophys. Acta Gene Regul. Mech. 2018, 1861, 338–343. [Google Scholar] [CrossRef]
  89. Schlaitz, A.L.; Thompson, J.; Wong, C.C.; Yates, J.R., 3rd; Heald, R. REEP3/4 ensure endoplasmic reticulum clearance from metaphase chromatin and proper nuclear envelope architecture. Dev. Cell 2013, 26, 315–323. [Google Scholar] [CrossRef]
  90. Burke, B. PREEParing for mitosis. Dev. Cell 2013, 26, 221–222. [Google Scholar] [CrossRef]
  91. Urlaub, H.; Raker, V.A.; Kostka, S.; Luhrmann, R. Sm protein-Sm site RNA interactions within the inner ring of the spliceosomal snRNP core structure. EMBO J. 2001, 20, 187–196. [Google Scholar] [CrossRef]
  92. Decker, C.J.; Parker, R. P-bodies and stress granules: Possible roles in the control of translation and mRNA degradation. Cold Spring Harb. Perspect. Biol. 2012, 4, a012286. [Google Scholar] [CrossRef]
  93. Irimia, M.; Rukov, J.L.; Penny, D.; Roy, S.W. Functional and evolutionary analysis of alternatively spliced genes is consistent with an early eukaryotic origin of alternative splicing. BMC Evol. Biol. 2007, 7, 188. [Google Scholar] [CrossRef]
  94. Cardoso, B.R.; Roberts, B.R.; Bush, A.I.; Hare, D.J. Selenium, selenoproteins and neurodegenerative diseases. Metallomics 2015, 7, 1213–1228. [Google Scholar] [CrossRef]
  95. Ding, W.; Wang, S.; Gu, J.; Yu, L. Selenium and human nervous system. Chin. Chem. Lett. 2023, 34, 108043. [Google Scholar] [CrossRef]
  96. Hayashi, S.; McMahon, A.P. Efficient recombination in diverse tissues by a tamoxifen-inducible form of Cre: A tool for temporally regulated gene activation/inactivation in the mouse. Dev. Biol. 2002, 244, 305–318. [Google Scholar] [CrossRef] [PubMed]
  97. Eckardt, D.; Theis, M.; Doring, B.; Speidel, D.; Willecke, K.; Ott, T. Spontaneous ectopic recombination in cell-type-specific Cre mice removes loxP-flanked marker cassettes in vivo. Genesis 2004, 38, 159–165. [Google Scholar] [CrossRef] [PubMed]
  98. Chakravarthy, S.; Keck, T.; Roelandse, M.; Hartman, R.; Jeromin, A.; Perry, S.; Hofer, S.B.; Mrsic-Flogel, T.; Levelt, C.N. Cre-dependent expression of multiple transgenes in isolated neurons of the adult forebrain. PLoS ONE 2008, 3, e3059. [Google Scholar] [CrossRef] [PubMed]
  99. Senserrich, J.; Batsivari, A.; Rybtsov, S.; Gordon-Keylock, S.; Souilhol, C.; Buchholz, F.; Hills, D.; Zhao, S.; Medvinsky, A. Analysis of Runx1 Using Induced Gene Ablation Reveals Its Essential Role in Pre-liver HSC Development and Limitations of an In Vivo Approach. Stem Cell Rep. 2018, 11, 784–794. [Google Scholar] [CrossRef]
  100. Crawley, J.N. Behavioral phenotyping strategies for mutant mice. Neuron 2008, 57, 809–818. [Google Scholar] [CrossRef]
  101. Kwon, D.Y.; Xu, B.; Hu, P.; Zhao, Y.T.; Beagan, J.A.; Nofziger, J.H.; Cui, Y.; Phillips-Cremins, J.E.; Blendy, J.A.; Wu, H.; et al. Neuronal Yin Yang1 in the prefrontal cortex regulates transcriptional and behavioral responses to chronic stress in mice. Nat. Commun. 2022, 13, 55. [Google Scholar] [CrossRef]
  102. Mastwal, S.; Li, X.; Stowell, R.; Manion, M.; Zhang, W.; Kim, N.S.; Yoon, K.J.; Song, H.; Ming, G.L.; Wang, K.H. Adolescent neurostimulation of dopamine circuit reverses genetic deficits in frontal cortex function. Elife 2023, 12, RP87414. [Google Scholar] [CrossRef]
  103. Bish, R.; Cuevas-Polo, N.; Cheng, Z.; Hambardzumyan, D.; Munschauer, M.; Landthaler, M.; Vogel, C. Comprehensive Protein Interactome Analysis of a Key RNA Helicase: Detection of Novel Stress Granule Proteins. Biomolecules 2015, 5, 1441–1466. [Google Scholar] [CrossRef]
  104. Shah, S.; Molinaro, G.; Liu, B.; Wang, R.; Huber, K.M.; Richter, J.D. FMRP Control of Ribosome Translocation Promotes Chromatin Modifications and Alternative Splicing of Neuronal Genes Linked to Autism. Cell Rep. 2020, 30, 4459–4472.e6. [Google Scholar] [CrossRef]
  105. Brown, A.L.; Wilkins, O.G.; Keuss, M.J.; Kargbo-Hill, S.E.; Zanovello, M.; Lee, W.C.; Bampton, A.; Lee, F.C.Y.; Masino, L.; Qi, Y.A.; et al. TDP-43 loss and ALS-risk SNPs drive mis-splicing and depletion of UNC13A. Nature 2022, 603, 131–137. [Google Scholar] [CrossRef]
  106. Takayama, K.I.; Suzuki, T.; Sato, K.; Saito, Y.; Inoue, S. Cooperative nuclear action of RNA-binding proteins PSF and G3BP2 to sustain neuronal cell viability is decreased in aging and dementia. Aging Cell 2024, 23, e14316. [Google Scholar] [CrossRef] [PubMed]
  107. Goebbels, S.; Bormuth, I.; Bode, U.; Hermanson, O.; Schwab, M.H.; Nave, K.A. Genetic targeting of principal neurons in neocortex and hippocampus of NEX-Cre mice. Genesis 2006, 44, 611–621. [Google Scholar] [CrossRef] [PubMed]
  108. Yang, X.; Yang, Y.; Sun, B.F.; Chen, Y.S.; Xu, J.W.; Lai, W.Y.; Li, A.; Wang, X.; Bhattarai, D.P.; Xiao, W.; et al. 5-methylcytosine promotes mRNA export—NSUN2 as the methyltransferase and ALYREF as an m(5)C reader. Cell Res. 2017, 27, 606–625. [Google Scholar] [CrossRef]
  109. Chen, X.; Li, A.; Sun, B.F.; Yang, Y.; Han, Y.N.; Yuan, X.; Chen, R.X.; Wei, W.S.; Liu, Y.; Gao, C.C.; et al. 5-methylcytosine promotes pathogenesis of bladder cancer through stabilizing mRNAs. Nat. Cell Biol. 2019, 21, 978–990. [Google Scholar] [CrossRef] [PubMed]
  110. Chaudhary, N.; McMahon, C.; Blobel, G. Primary structure of a human arginine-rich nuclear protein that colocalizes with spliceosome components. Proc. Natl. Acad. Sci. USA 1991, 88, 8189–8193. [Google Scholar] [CrossRef]
  111. Twyffels, L.; Gueydan, C.; Kruys, V. Shuttling SR proteins: More than splicing factors. FEBS J. 2011, 278, 3246–3255. [Google Scholar] [CrossRef]
  112. Zhang, W.J.; Wu, J.Y. Functional properties of p54, a novel SR protein active in constitutive and alternative splicing. Mol. Cell Biol. 1996, 16, 5400–5408. [Google Scholar] [CrossRef] [PubMed]
  113. Kennedy, C.F.; Kramer, A.; Berget, S.M. A role for SRp54 during intron bridging of small introns with pyrimidine tracts upstream of the branch point. Mol. Cell Biol. 1998, 18, 5425–5434. [Google Scholar] [CrossRef] [PubMed]
  114. Gehring, N.H.; Roignant, J.Y. Anything but Ordinary—Emerging Splicing Mechanisms in Eukaryotic Gene Regulation. Trends Genet. 2021, 37, 355–372. [Google Scholar] [CrossRef]
Figure 1. Structures of the murine Ataxin-2-like protein and gene. (A) Scheme of the ATXN2L protein domains (not depicted to scale), with the experimentally verified 1049 amino acid sequence above, and 3 predicted protein isoforms below. The reported Proline-rich, MPL-binding, Lsm, LsmAD, and PAM2 interaction motifs are shown in their positions relative to the coding exons, which are illustrated as red and yellow cylinders. Red lines highlight the differences between isoforms. (B) Scheme of the Atxn2l gene (not depicted to scale), with its endogenous allele above, versus its recombined allele below. Gray boxes: Atxn2l coding exons. Solid lines: intronic/intergenic regions. Gray arrow: neomycin (neo) as positive-selection cassette flanked by RoxP recombination sites (orange rhombuses) for in vivo excision. Blue triangles: loxP sites. Yellow box: diphtheria toxin fragment A (DTA) as a negative selection marker. Primer names and orientations are shown as colored arrows, with nucleotide numbers reflecting distance from the 126115977 end in genomic clone NC_000073.7.
Figure 1. Structures of the murine Ataxin-2-like protein and gene. (A) Scheme of the ATXN2L protein domains (not depicted to scale), with the experimentally verified 1049 amino acid sequence above, and 3 predicted protein isoforms below. The reported Proline-rich, MPL-binding, Lsm, LsmAD, and PAM2 interaction motifs are shown in their positions relative to the coding exons, which are illustrated as red and yellow cylinders. Red lines highlight the differences between isoforms. (B) Scheme of the Atxn2l gene (not depicted to scale), with its endogenous allele above, versus its recombined allele below. Gray boxes: Atxn2l coding exons. Solid lines: intronic/intergenic regions. Gray arrow: neomycin (neo) as positive-selection cassette flanked by RoxP recombination sites (orange rhombuses) for in vivo excision. Blue triangles: loxP sites. Yellow box: diphtheria toxin fragment A (DTA) as a negative selection marker. Primer names and orientations are shown as colored arrows, with nucleotide numbers reflecting distance from the 126115977 end in genomic clone NC_000073.7.
Cells 14 01532 g001
Figure 2. (AD) Experimental design to cross Atxn2l-floxed mice with CamK2a-Cre/ER2 transgenic mice, administer tamoxifen, and control deletion success using genotypes at the DNA and RNA levels. (A) Planned crossbreeding and genotypes of Atxn2l-cKO and control mice. Mice were aged 2–3 months, injected with tamoxifen (TAM) over 5 consecutive days, subjected to locomotor phenotyping until the age of 9 months, and then had tissue collected for immunohistochemistry and proteomic analysis. (B) Experimental timeline. (C) DNA from ear punches of Atxn2l-flox hom/Cre-WT and Atxn2l-flox hom/Cre-Tg, both treated with TAM; different control mice were analyzed for the floxed locus, Cre presence, and successful Atxn2l deletion through efficient Cre expression. (D) RNA from frontal cortex tissue of Atxn2l-flox hom/Cre-WT and Atxn2l-flox hom/Cre-Tg, both treated with TAM; control mice were analyzed for successful Atxn2l deletion with SYBR Green technology using RT-qPCR. Primer details are provided in Table S1.
Figure 2. (AD) Experimental design to cross Atxn2l-floxed mice with CamK2a-Cre/ER2 transgenic mice, administer tamoxifen, and control deletion success using genotypes at the DNA and RNA levels. (A) Planned crossbreeding and genotypes of Atxn2l-cKO and control mice. Mice were aged 2–3 months, injected with tamoxifen (TAM) over 5 consecutive days, subjected to locomotor phenotyping until the age of 9 months, and then had tissue collected for immunohistochemistry and proteomic analysis. (B) Experimental timeline. (C) DNA from ear punches of Atxn2l-flox hom/Cre-WT and Atxn2l-flox hom/Cre-Tg, both treated with TAM; different control mice were analyzed for the floxed locus, Cre presence, and successful Atxn2l deletion through efficient Cre expression. (D) RNA from frontal cortex tissue of Atxn2l-flox hom/Cre-WT and Atxn2l-flox hom/Cre-Tg, both treated with TAM; control mice were analyzed for successful Atxn2l deletion with SYBR Green technology using RT-qPCR. Primer details are provided in Table S1.
Cells 14 01532 g002
Figure 3. Mosaic depletion of ATXN2L protein in the frontal cortex of Atxn2l-flox/CamK2a-CreERT2 mice after TAM application (cKO). (A) Overview images of ATXN2L staining in the frontal cortex at different distances from the bregma. A reduction in the number of stained cells in a cKO mouse (right) compared with a control animal (left) is visible. (B) Higher magnification of a portion of the frontal cortex stained for both ATXN2L and CamK2a. In the control brain, virtually all neurons that are positive for CamK2a also express ATXN2L. ATXN2L staining that does not colocalize with CamK2a staining likely represents ATXN2L in interneurons and glial cells. In the cKO brain, a mosaic deletion of ATXN2L in CamK2a-expressing neurons can be observed. Filled arrows point to examples of CamK2a-positive cells that have lost ATXN2L presence.
Figure 3. Mosaic depletion of ATXN2L protein in the frontal cortex of Atxn2l-flox/CamK2a-CreERT2 mice after TAM application (cKO). (A) Overview images of ATXN2L staining in the frontal cortex at different distances from the bregma. A reduction in the number of stained cells in a cKO mouse (right) compared with a control animal (left) is visible. (B) Higher magnification of a portion of the frontal cortex stained for both ATXN2L and CamK2a. In the control brain, virtually all neurons that are positive for CamK2a also express ATXN2L. ATXN2L staining that does not colocalize with CamK2a staining likely represents ATXN2L in interneurons and glial cells. In the cKO brain, a mosaic deletion of ATXN2L in CamK2a-expressing neurons can be observed. Filled arrows point to examples of CamK2a-positive cells that have lost ATXN2L presence.
Cells 14 01532 g003
Figure 4. Phenotype progression in an open field paradigm, showing the parameter “ambulatory time” with mean values and variance as SEM, as well as linear regression lines. All animals studied were injected with tamoxifen, but only flox/Cre mice (n = 7–9) could produce a cKO in CamK2a+ neurons and have subsequent movement deficits, while Atxn2l-flox/Cre-Tg and Atxn2l-flox/Cre-WT mice (n = 5–6) are expected to recover normal movement activity over time.
Figure 4. Phenotype progression in an open field paradigm, showing the parameter “ambulatory time” with mean values and variance as SEM, as well as linear regression lines. All animals studied were injected with tamoxifen, but only flox/Cre mice (n = 7–9) could produce a cKO in CamK2a+ neurons and have subsequent movement deficits, while Atxn2l-flox/Cre-Tg and Atxn2l-flox/Cre-WT mice (n = 5–6) are expected to recover normal movement activity over time.
Cells 14 01532 g004
Figure 5. Volcano plot illustrating relevant dysregulations in the global proteome of the frontal cortexes of Atxn2l-cKO mice. A –log10 (p-value) of 1.3 corresponds to a p-value of 0.05 as the threshold for nominal significance; a log2 (fold-change) of −0.41 reflects the depletion of the ATXN2L protein. Factors with stronger downregulations are visualized as blue dots with gene symbols, with stronger upregulations in red and weaker dysregulations in purple.
Figure 5. Volcano plot illustrating relevant dysregulations in the global proteome of the frontal cortexes of Atxn2l-cKO mice. A –log10 (p-value) of 1.3 corresponds to a p-value of 0.05 as the threshold for nominal significance; a log2 (fold-change) of −0.41 reflects the depletion of the ATXN2L protein. Factors with stronger downregulations are visualized as blue dots with gene symbols, with stronger upregulations in red and weaker dysregulations in purple.
Cells 14 01532 g005
Table 1. Offspring counts. After crossing with constitutive Cre-deleter mice, Atxn2l+/− intercrosses produce offspring with postnatal genotype distribution that confirms embryonic lethality upon homozygous exon 10–17 deletion.
Table 1. Offspring counts. After crossing with constitutive Cre-deleter mice, Atxn2l+/− intercrosses produce offspring with postnatal genotype distribution that confirms embryonic lethality upon homozygous exon 10–17 deletion.
Observed/Expected Number of Live Born Mice with Indicated Genotype
+/++/−−/−Number of Offspring
Live born female33/2739/540/2772/108
Live born male20/2726/540/2746/108
Live born total53/5465/1080/54118/216
Disclaimer/Publisher’s Note: The statements, opinions and data contained in all publications are solely those of the individual author(s) and contributor(s) and not of MDPI and/or the editor(s). MDPI and/or the editor(s) disclaim responsibility for any injury to people or property resulting from any ideas, methods, instructions or products referred to in the content.

Share and Cite

MDPI and ACS Style

Key, J.; Almaguer-Mederos, L.-E.; Kandi, A.R.; Fellenz, M.; Gispert, S.; Köpf, G.; Meierhofer, D.; Deller, T.; Auburger, G. Conditional ATXN2L-Null in Adult Frontal Cortex CamK2a+ Neurons Does Not Cause Cell Death but Restricts Spontaneous Mobility and Affects the Alternative Splicing Pathway. Cells 2025, 14, 1532. https://doi.org/10.3390/cells14191532

AMA Style

Key J, Almaguer-Mederos L-E, Kandi AR, Fellenz M, Gispert S, Köpf G, Meierhofer D, Deller T, Auburger G. Conditional ATXN2L-Null in Adult Frontal Cortex CamK2a+ Neurons Does Not Cause Cell Death but Restricts Spontaneous Mobility and Affects the Alternative Splicing Pathway. Cells. 2025; 14(19):1532. https://doi.org/10.3390/cells14191532

Chicago/Turabian Style

Key, Jana, Luis-Enrique Almaguer-Mederos, Arvind Reddy Kandi, Meike Fellenz, Suzana Gispert, Gabriele Köpf, David Meierhofer, Thomas Deller, and Georg Auburger. 2025. "Conditional ATXN2L-Null in Adult Frontal Cortex CamK2a+ Neurons Does Not Cause Cell Death but Restricts Spontaneous Mobility and Affects the Alternative Splicing Pathway" Cells 14, no. 19: 1532. https://doi.org/10.3390/cells14191532

APA Style

Key, J., Almaguer-Mederos, L.-E., Kandi, A. R., Fellenz, M., Gispert, S., Köpf, G., Meierhofer, D., Deller, T., & Auburger, G. (2025). Conditional ATXN2L-Null in Adult Frontal Cortex CamK2a+ Neurons Does Not Cause Cell Death but Restricts Spontaneous Mobility and Affects the Alternative Splicing Pathway. Cells, 14(19), 1532. https://doi.org/10.3390/cells14191532

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop