CLN3 Batten disease (CLN3 disease) is a pediatric lysosomal storage disorder that presents with progressive blindness, motor and cognitive decline, seizures, and premature death. CLN3 disease results from mutations in CLN3 with the most prevalent mutation, a 966 bp deletion spanning exons 7–8, affecting ~ 75% of patients. Mouse models with complete Cln3 deletion or Cln3Δex7/8 mutation have been invaluable for learning about both the basic biology of CLN3 and the underlying pathological changes associated with CLN3 disease. These models, however, vary in their disease presentation and are limited in their utility for studying the role of nonsense mediated decay, and as a consequence, in testing nonsense suppression therapies and read-through compounds. In order to develop a model containing a disease-causing nonsense point mutation, here we describe a first-of-its-kind Cln3Q352X mouse model containing a c.1054C > T (p.Gln352Ter) point mutation. Similar to previously characterized Cln3 mutant mouse lines, this novel model shows pathological deficits throughout the CNS including accumulation of lysosomal storage material and glial activation, and has limited perturbation in behavioral measures. Thus, at the molecular and cellular level, this mouse line provides a valuable tool for testing nonsense suppression therapies or read through compounds in CLN3 disease in the future.
CLN3 Batten disease (CLN3 disease), also referred to as juvenile neuronal ceroid lipofuscinosis (JNCL), is an autosomal recessive disorder caused by mutations in CLN3. It is the most common form of Batten disease with over 40 known pathogenic mutations in CLN31,2. Patients typically present with progressive vision loss starting around 5 years of age as well as advanced cognitive and motor decline, development of behavioral problems, seizures, and ultimately death3. The most prevalent disease causing CLN3 mutation, accounting for ~ 75% of all homozygous mutations and ~ 20% of compound heterozygous mutations, is a 966 bp deletion that deletes exons 7 and 84. Additionally, a broad spectrum of splice variants, missense, nonsense and frameshift mutations exist that result in non-syndromic retinal disease, protracted disease course, or the common CLN3 disease progression (reviewed in5). Rather than looking at a “one-size-fits-all” approach to therapies, researchers and clinicians are analyzing individual patient genetics to determine whether biologicals, read-through compounds or targeted genetic approaches, like gene therapy6 or antisense oligonucleotides7,8, can impact disease progression (See reviews9,3). Therefore in order to have translational success, it is paramount to have robust animal models in place to develop and test these prospective, tailored therapies of CLN3 disease.
Nonsense mediated decay (NMD) is an evolutionarily conserved quality control pathway in eukaryotic organisms that is responsible for inspecting mRNA for errors and eliminating any error-containing transcripts from the transcriptome, as well as controlling the amount of non-mutated transcript in the transcriptome10. NMD typically occurs during the first translation of mutant transcript, where mutant mRNAs that contain premature termination codons (PTC) prohibit the ribosome from reaching and removing the exon junction complex, ultimately triggering the NMD signaling cascade10. PTCs can be caused by various mutations, though nonsense point mutations are specifically characterized as creating a PTC through the mutation of a single base pair. Nonsense point mutations are frequent causes of human inherited diseases, accounting for approximately 20% of all disease-causing single base pair mutations11,12. While NMD is important for quality control, in the context of human disease NMD may exacerbate disease progression, as some truncated proteins’ partial function may be enough to mitigate or reduce the severity of the disease13. As such, NMD is a growing target for therapeutic intervention through the use of read-through compounds, which promote translation through the PTC, or nonsense suppression therapies, which block the NMD signaling cascade, in several disease indications, including Batten disease14,15.
Mouse models with complete Cln3 deficiency or carrying the common 966 bp deletion of exons 7 and 8 have been generated in order to better study and understand CLN3 disease16,17,20. While the Δ7/8 genotype results in a frameshift mutation, 28 novel amino acids, and a PTC18,19,20, the model is not suitable for exploring read-through compounds or nonsense suppression therapies, as the addition of 28 novel amino acids may generate a translated protein with altered function relative to wildtype Cln3. However, previous research in a nonsense point mutant CLN3 patient line (c.1054C > T (p.Gln352Ter)) revealed that CLN3Q352X mRNA expression could be increased via NMD inhibition by siRNA-mediated knockdown, opening the door to study the effects of nonsense suppression and read-through therapies using a relevant CLN3 point mutation.
Here, to expand on testing this therapeutic approach for CLN3 disease, we generated a novel, nonsense point mutant mouse model of CLN3 disease based on the CLN3 patient mutation described above. We report the molecular, behavioral and neuropathological characterization of homozygous Cln3Q352X mice, showcasing their utility as a model of CLN3 disease and potential for screening nonsense suppression and read-through therapies in the future.
Generation of Cln3 Q352X mice
Cln3Q352X mice were generated by Applied StemCell Inc. using CRISPR technology to introduce a nonsense mutation in exon 16 (CAG > TAG), causing glutamine352 (Q) to be replaced with a premature stop codon (X). Two Cln3 guide RNAs were selected (Table 1), cloned into guide RNA/cas9 expression vectors, and transfected into mouse N2A cells for evaluation of non-homologous end joining efficiency (Fig. 1A,B). While mCLN3.g13 had greater efficiency (37% vs. 21%), mCLN3.g14 was chosen to generate donor DNA due to its optimal position to the point mutation.
A single stranded oligodeoxylnucleotide donor was made based on mCLN3.g14, with a silent mutation added to leucine351 (CTC > TTG) to prevent the repaired genome sequence from being re-targeted, and combined with mCLN3.g14 Cas-9 vectors and active guide RNA (Fig. 1C). The mCln3-Q352X CRISPR cocktail was injected into the cytoplasm of C57BL/6 embryos, and newborn mice screened for integration. Of the 100 embryos injected, 76 developed and were implanted into three surrogate mice, with 12 mice ultimately born. One cloned male was heterozygous for the Cln3Q352X mutation and one male was homozygous, as confirmed by sequencing chromatograms (Fig. 1D, homozygous animal). These two animals were used as founders and mated to wildtype females to produce the F1 generation, which produced nine male and four female heterozygous Cln3Q352X animals that were sequenced, shipped, and bred to generate homozygous Cln3Q352X mice (Fig. 1E, heterozygous founder).
Cln3 Q352X mice show reduced Cln3 transcript levels and variable TPP1 and PPT1 enzyme activities
mRNA was measured in various tissues from wildtype and Cln3Q352X mice to determine Cln3 transcript levels. Significantly different Cln3Q352X transcript levels ranged from 34 to 67% of wildtype and were seen in several tissues of both male and female Cln3Q352X mice, including the cerebral cortex, thalamus, brainstem, lung, and kidney (Table 2). Cln3Q352X males also had lower transcript levels in the spleen and liver, whereas Cln3Q352X female mice displayed decreased transcript levels in the heart and eye.
Loss of CLN3 has been shown to affect lysosomal function21,22,23, and several recent articles have shown that various lysosomal enzymes, including PPT1 (protein product of CLN1) and TPP1 (protein product of CLN2), are altered in Cln3Δ7/8 mice24,25. To examine whether this was the case in Cln3Q352X mice, PPT1 and TPP1 enzyme activity assays were performed, showing decreased PPT1 activity in the liver of Cln3Q352X mice and increased TPP1 activity in the thalamus and cerebellum (Table 2), consistent with previous reports26,27.
Cln3 Q352X mice have typical pathological progression of Batten disease hallmarks
Wildtype and homozygous Cln3Q352X mice were sacrificed at 6 and 21 months of age (early and late disease stage) to determine whether the mouse model displayed the typical pathological progression reported in CLN3 patients and other Cln3 models. In particular, astrocyte activation (GFAP+), microgliosis (CD68+), and accumulation of lysosomal storage material (mitochondrial ATP synthase subunit C) were examined in the brain as hallmarks of CLN3 disease progression28,29,30,31,32. As regional pathogenesis starts in the somatosensory cortex and thalamus, and male and female patients have shown differences in disease progression, assays were analyzed across gender in the somatosensory barrel field (S1BF) cortex and the ventral posteromedial/ventral posterolateral (VPM/VPL) nuclei of the thalamus4,33.
At 6 months, subunit C accumulation was already significantly present in both the S1BF and the VPM/VPL of Cln3Q352X mice while wildtype controls showed extremely minor amounts of positive immunoreactivity (Fig. 2A). Astrocytosis was also prominent at 6 months with females showing increased values in the S1BF (Fig. 2B). Additionally, there were qualitative differences in astrocyte morphology between wildtype and Cln3Q352X mice, with Cln3Q352X astrocytes appearing slightly more hypertrophic and ramified. There was no significant difference, however, in microglial activation at this early 6 month timepoint (Fig. 2C). Pathology was widespread and significantly exemplified at 21 months, which is near end stage of a normal mouse lifespan. Subunit C accumulation was evident throughout the brain, increasing in both S1BF and VPM/VPL regions with no apparent sex differences (Fig. 3A). Astrocytosis followed a similar trend in both regions with obvious differences in morphology as Cln3Q352X displayed extreme hypertrophy and ramification when compared to wildtype animals(Fig. 3B). Additionally, microglial activation was significantly elevated in Cln3Q352X mice at 21 months in the VPM/VPL for both sexes while only males were significantly altered in the S1BF compared to their wild type counterparts (Fig. 3C).
Behavioral evaluation of Cln3 Q352X mice reveals sex-dependent motor coordination deficits
While other Cln3 mouse models are notorious for their limited and inconsistent behavior deficits, we sought to thoroughly characterize any motor coordination deficits that may be present in Cln3Q352X mice. When assessed on an accelerated rotarod test, Cln3Q352X mice generally performed similarly to their wild type counterparts, and in some instances performed better compared to wild type mice (Fig. 4A). When assessed for motor coordination deficits using another assay, a modified vertical descent test, male Cln3Q352X mice showed significant difficulties in climbing down and turning down the pole (Fig. 4B,C). These deficits were prominent from 3 months of age, with wild type males performing poorly at the test as they aged. Female Cln3Q352X mice, however, showed inconsistent deficits in these assays.
Lastly, in order to control for weight and anxiety as confounding factors in behavior results, mice were weighed at each time point and subjected to a light–dark test to assess their preference for dark areas. Cln3Q352X male mice weighed less than their wildtype cohorts at 3, 6 and 18 months, while Cln3Q352X female mice weighed less only at 6 months (Fig. 4D). Any weight disadvantages experienced by wildtype mice would be most prominent at these time points, which is not seen in the rotarod test, as there were no differences between wildtype and Cln3Q352X mice at these time points. However, heavier wildtype mice may have been disadvantaged in the 18 month vertical descent test, as male wildtype mice took significantly longer to descend the pole when compared to the lighter Cln3Q352X male mice. When assessed for anxiety and preference for dark areas, both groups spent the majority of their time in the dark side of the box with only one significant difference in female Cln3Q352X mice at 1 month of age (Fig. 4E), indicating that anxiety likely did not contribute to the results of the other behavioral tests.
Batten disease is a lysosomal storage disorder that, while individual subtypes are rare, represents the most common pediatric neurodegenerative disease worldwide. CLN3 Batten disease results from homozygous mutations in CLN3, which are present in ~ 80% of individuals inflicted with Batten disease. Although the function of the CLN3 protein is unknown, the pathogenic progression of the disease is well established in both human patients and animal models. Common symptoms of CLN3 Batten disease include progressive vision loss, neurocognitive decline, behavioral changes, and motor deficit with symptom onset beginning around ~ 4–8 years and death occurring at ~ 20 years. In mouse models of CLN3 Batten disease, disease progression results in whole brain atrophy, including region-specific atrophy in the cortex, hippocampus, thalamus, and cerebellum. Additionally, mice present with pathological hallmarks including reactive gliosis, neuroinflammation, and accumulation of ASM. However, while Cln3 mouse models recapitulate some motor and pathological signs of the disease, the visual and cognitive aspects of the disease in human patients do not develop.
While the genetic knockout mouse models have been beneficial for studying the selective pathogenesis of Batten disease, recently, tailored mouse models have been generated to develop therapies to individual mutations. Generation of novel mouse models from patient mutations of Batten disease present with many of the same neuronal and visual phenotypes seen in patients29,31,34,35,36,37,38,39,40,41,42,43,44,45,46,47,48,49,50,51,52,53,54,55,56,57,58,59. Regional-specific vulnerability of cortical, hippocampal, thalamic, and cerebellar regions of the CNS have been identified in many of the murine models of Batten disease29,31,37,38,44,60,61. These models also help in longitudinal identification of pathological hallmarks and detection of glial activation before neuronal changes occur.
Cln3Q352X displayed the typical pathological progression of disease hallmarks as other Cln3 mouse models. ASM was evident in the somatosensory cortex and the thalamus as early as 6 months (Fig. 2A) and became widespread and extreme at 21 months of age (Fig. 3A). Similarly, reactive astrocytosis was prevalent at 6 months (Fig. 2B) which significantly worsened at 21 months with clear morphological differences between wild type and Cln3Q352X mice (Fig. 3B). While microglial activation (CD68) at 6 months was not significant in either of the brain regions analyzed, it was significantly increased at 21 months in Cln3Q352X mice, and it Cln3Q352X mice appeared to have hypertrophic microglia at this stage in disease (Fig. 3C).
We have previously demonstrated that the neurological deficits in the Cln3-/- and Cln3Δex7/8 mouse models of juvenile CLN3 disease strongly depend on the genetic background and gender 34, and female CLN3 patients have reported more severe symptoms33. Therefore, the age-dependent disparate behavioral test results of male and female Cln3Q352X mice are not surprising, though notably female Cln3Q352X mice lacked a consistent, more severe phenotype. In the vertical pole test, Cln3Q352X mice showed age dependent motor deficits compared to wild type mice. In the accelerating rotarod test, however, Cln3Q352X mice performed better than wild type mice at certain ages. These surprising results are not unique to Cln3Q352X mice, as we have previously shown that while Cln3Δex7/8 female mice displayed motor deficits in the vertical pole test, they performed markedly better than their wild type and Cln3−/− counterparts in the rotarod test34.
Although, decreased Cln3Q352X transcript levels were seen in several organs and brain regions of both male and female Cln3Q352X mice (Table 2), no statistically significant reduction of Cln3Q352X mRNA was detected in the cerebellum, muscle, heart and eye of males, and the cerebellum, muscle, spleen and liver of females. It has been shown that inter-tissue and sex variations exist in the efficiency of nonsense-mediated mRNA decay in mice, and therefore, it is possible that these variations account for the differences seen in our model62,63. It has previously been shown that the activity of the soluble lysosomal enzyme, TPP1 (product of the CLN2 gene) is markedly increased in the brain of patients with juvenile CLN3 disease and also in the brain of Cln3-/- mice24,25,26. In Cln3Q352X mice, however, TPP1 activity, was only significantly elevated in the thalamus and cerebellum, perhaps suggesting that the Cln3Q352X mutation does not affect lysosomal function as severely as the most common disease-causing deletion (Cln3Δex7/8) or the complete lack of Cln3 (Cln3-/-). Importantly, the clinical presentation of the Cln3Q352X patient mutation has not been reported, and it is therefore unclear whether the point mutation brings about less severe cellular manifestations and, as a consequence, disease course.
Taken together, we show pathological and behavioral characterization of a novel point mutant Cln3Q352X mouse model, which shows progression of pathological symptoms similar to the common Cln3Δex7/8 mouse model. Beneficially, Cln3Q352X model enables the screening of read-through and nonsense suppression therapies in the future, that if tested in the common Cln3Δex7/8 model would be confounded by the presence of novel amino acids. Therefore, this novel model shows its utility as a pathological model of CLN3 Batten disease, and its potential as a tool for screening tailored genetic therapies in the future.
All animal research performed for this manuscript followed National Institute of Health (NIH) and Sanford Research Institutional Animal Care and Use Committee (IACUC) guidelines. The animal protocol for this study was reviewed and approved by the Sanford Research IACUC.
Cln3Q352X mice were generated by Applied StemCell Inc. (CA). Using CRISPR technology, a nonsense mutation was introduced in exon 16 (CAG > TAG) causing glutamine352 (Q) to be replaced with a premature stop codon. Addition of a silent mutation (CTC > TTG) directly before the nonsense mutation was necessary to generate the mouse line and codes for the same amino acid (leucine). Specific guide RNAs, oligo donors, and Cas-9 vectors are described in Fig. 1 and Table 1. gRNA non-homologous end joining efficiency was determined by Applied StemCell Inc. using a SURVEYOR assay on PCR products (Transgenomic Inc., #706020), and cloned and F1 generations were confirmed by sequencing chromatograms. F2 generations were sequence confirmed using a quantitative real-time polymerase chain reaction assay (Forward primer: 5′- ACGGTTCACCTGGGTCCTA-3′; Reverse primer: 5′-GAGGTGGGTGTGAACAAACAG-3′; Reporter 1(VIC): 5′-CACTCAGTACCTGGAGCAG-3′; Reporter 2(FAM): 5′- CACTCAGTACCTACAACAG-3′) from Thermo Fisher Scientific. Thermal profile for qRT-PCR assay included: 1) 95 °C for 15 min. (1 cycle) and 2) 95 °C for 15 s. and 60 °C for 1 min. (40 cycles). Cln3Q352X mice were generated and maintained on the C57BL/6J (Stock #000664) background and were characterized in comparison to wild type C57BL/6J mice maintained in our mouse colony. All mice were housed, cared for, and used under the procedures developed by the NIH and the direction of the Sanford Research IACUC (Protocol #: 129-03-20B). Mice were housed in separately vented microisolator cages (maximum of five mice per cage) with access to food and water without restrictions, with the room maintained at a 14 h dark: 10 h light cycle. Mice were fed with the Teklad Global 2918 diet (Harlan Laboratories, IN) and their drinking water was tap water.
All behavior tests were performed during the 10 h light cycle. Mice performed three different tests to determine the impact of the Cln3Q352X mutation on parameters of performance such as motor coordination, spatial awareness, and anxiety-like behavior. Mice were divided into two behavioral cohorts to minimize motor learning and repeated measures testing. Behavioral tests were performed on the same groups of male and female Cln3Q352X mice and wild type mice in Cohort 1: 1, 3, and 6 months of age (n = 12 /sex/genotype) and Cohort 2: 9, 12, and 18 months of age (n = 11 of each sex/genotype). Before behavioral tests were performed, mice were allowed a 20 min acclimation period to their testing environment.
Motor coordination was assessed using an accelerating rotarod test as previously described64. In brief, a Rota Rod Rotamex-5 (Columbus Instruments, OH) was utilized. Parameters for the rotarod test were as follows: start speed: 0 rotations per minute (rpm); end speed: 48 rpm, acceleration: 0.2 rpm per second, and total allotted test time: 240 s. Mice underwent three consecutive training runs on the rotarod before a 1.5 h rest period. After the rest period, mice were tested on the rotarod for three test trials comprising three consecutive testing runs with 15 min of rest between each trial. Latency to fall was analyzed as an average of the nine test runs for each mouse.
Modified vertical pole test
In order to test motor coordination and spatial awareness, a modified vertical pole test was performed as previously described64. Briefly, the vertical pole utilized a threaded metal pole attached to a padded base and consisted of two tests: (1) climb down: mice were placed at the top of the and timed until they climbed down to the base of the; and (2) turn downward: mice were placed at the top of the pole facing up and timed until they turn downward. For the climb down test, mice were given 60 s to climb down the pole, performing the test five consecutive times. During the turn downward test, mice were again given 60 s to turn around and face downward, performing the test four consecutive times. Mice that fall off the pole in either test were given a score of 60 s. The total sum of time in the trials for each test and for each mouse was calculated for analysis.
Mice were placed individually into a box with a light side and a dark side (Stoelting Co., IL) and allowed to roam freely for 10 min. Mouse movement was recorded and tracked using ANYmaze equipment and software (Stoelting Co., IL). Software data was used to determine the amount of time spent in each area of the box. The time spent in the dark box is proportional to anxiety, as anxious mice spend little time in the light box.
Tissue collection and preparation
For enzyme analysis and transcript abundance, Cln3Q352X mice and wild type mice (n = 4/sex/genotype) were euthanized using a carbon dioxide chamber at 1 month of age. Following euthanasia, mice were flushed with 10 ml of sterile phosphate buffered saline solution by cardiac perfusion. Collected tissues were flash frozen on dry ice, and included the cerebral cortex, cerebellum, striatum/thalamus, liver, and kidney. All flash frozen tissues were stored at − 80 °C until analysis. Tissues for enzyme analysis were homogenized, processed, and extracted using a Maxwell 16 LEV simplyRNA tissue kit (Promega), while tissues for enzyme analysis were homogenized in protein lysis buffer. Homogenization of tissues was performed in a Bertin Technologies Precellys 24 homogenizer using 2-ml tubes containing zirconium beads. For histological analysis, Cln3Q352X mice and wild type mice (n = 6/sex/genotype) were euthanized at 6 and 21 months of age. Following euthanasia, animals were flushed with 10 ml of sterile phosphate buffered saline solution followed by a 10-ml perfusion of 4% paraformaldehyde in PBS both via cardiac perfusion. Extracted brains were placed into scintillation vials containing 4% paraformaldehyde in PBS. Brains were stored at 4 °C with PBS containing 0.02% sodium azide replacing the 4% paraformaldehyde solution after 24 h fixation. Brains were set in 5% low melting agarose and sliced coronally into 50 μm sections using a Leica VT1000S vibratome in a 1:6 serial collection.
Protein sample preparation
Protein sample preparation was performed as previously described27. Briefly, tissue were cut and placed into 2-ml tubes containing zirconium beads and 500 μl of protein lysis buffer and homogenized using a Bertin Technologies Precellys 24 homogenizer. Homogenized samples were centrifuged at 12,000g for 10 min with supernatant sample transfered to 1.5-ml microcentrifuge tubes and storage at − 80 °C. Total protein concentrations were determined using the Pierce 660 nm Protein Assay (Thermo Fisher Scientific).
Batten-related lysosomal enzyme activity assays
Evaluation of TPP1 (tripeptidyl peptidase 1) and PPT1 (palmitoyl protein transferase 1) enzyme activities were completed using samples from Cln3Q352X and wild type mice as previously described14,27. Assays were performed on 10 μg of protein sample per well. For the TPP1 enzyme assay, protein sample was accompanied by 40 μl of 250 μM Ala-Ala-Phe-7-amido-4-methylcoumarin diluted in substrate buffer (150 mM NaCl; 0.1% Triton X-100; 100 mM sodium acetate; pH 4.0). PPT1 enzyme assay included protein sample accompanied by 20 μl of PPT1 substrate (0.64 mM 4-methylumbelliferyl-6-thiopalmitoyl-β-glucoside; 15 mM dithiothreitol with 2.3 mg/ml bovine serum albumin and 0.09% sodium azide; 0.2 M disodium phosphate with 0.1 M citric acid buffer; 0.945 mg/ml β-glucosidase; pH 4.0). Enzyme activity assay plates were incubated in the dark for 1 h at 37 °C, then 200 μl of stop buffer was added (TPP1 Stop Buffer: 0.1 M monochloroacetic acid, 0.13 M NaOH, 0.1 M acetic acid, pH 4.3; PPT1 Stop Buffer: 0.5 M sodium bicarbonate with 0.5 M sodium carbonate, 0.025% Triton X-100, pH 10.7). Fluorescence was measured using a BioTek Cytation 3 (TPP1: Excite 380 nm/Emit 460 nm; PPT1: Excite 355 nm/Emit 460 nm). With background fluorescence being accounted for, relative fluorescence was measured as a percentage of wild type fluorescence.
RNA sample preparation and reverse transcription for cDNA synthesis
RNA and cDNA sample preparation were performed as previously described27. RNA sample concentrations were calculated and cDNA synthesis was executed on 1 μg of total RNA using GoScript Reverse Transcription System (Promega). RT-PCR Reactions were performed on an Applied Biosystems Veriti Thermal Cycler according to manufacturer’s protocol. Samples were stored at − 20 °C.
Quantitative polymerase chain reaction
Using nuclease-free water, cDNA samples were diluted 1:20. Quantitative polymerase chain reactions were performed using Absolute Blue Q-PCR Mix (Thermo Fisher Scientific). Cln3 (Forward primer: 5′-TGGAGACCAGTGACAAGCA-3′; Reverse primer: 5′-TCAAGGGAGGTGACAGAGGA-3′) and Gapdh expression (Forward primer: 5′-ACCACAGTCCATGCCATCAC-3′; Reverse primer: 5′-TCCACCACCCTGTTGCTGTA-3′) were quantified. Reactions were performed in a Stratagene Mx3005P (Agilent Technologies) under the following conditions: 1) 95 °C for 15 min. (1 cycle) and 2) 95 °C for 15 s.; 60 °C for 1 min. (40 cycles). 2-ΔΔCT method was used to analyze relative fold expression65.
Three brain sections per animal were selected to contain the ventral posteromedial (VPM)/ventral posterolateral (VPL) nuclei of the thalamus and the somatosensory barrel field (S1BF) cortex. Immunohistochemistry was performed as previously described66. Briefly, free floating brain sections were incubated in 1% hydrogen peroxide in Tris-buffered saline (TBS) for 20 min to block endogenous peroxidase activity followed by 3 washes in TBS. Sections were then blocked in 15% goat serum-containing TBS-T (TBS with 0.3% Triton X-100) for 30 min followed by primary antibody solution overnight at 4 °C. Primary antibodies included: anti-CD68 (BioRad AbD Serotec, MCA1957; 1:2,000), anti-GFAP (Dako, Z0334; 1:8,000), and anti-ATP synthase C (Abcam, ab181243, 1:1,000) diluted in TBS-T+ 10% goat serum. Secondary antibodies included: biotinylated anti-rat and anti-rabbit IgGs (Vector Labs, BA-9400, BA-1000; 1:2000) diluted in TBS-T+ 10% goat serum. An ABC amplification kit (Vector Labs) was used for 2 h followed by 0.05% DAB solution until visible reaction had occurred.
Image acquisition and analysis
All microscope slides were scanned on a Leica DM6000B slide scanning microscope at 20X. Images were extracted in 2,400 × 2,400 pixel fields from appropriate regions and analyzed using an image threshold analysis using ImageJ (version 1.51). High-resolution images for figures were taken on a Nikon NiE microscope.
Statistical analyses were performed using GraphPad Prism (v6.04). Male and female Cln3Q352X mice were compared to their same-sex cohort for all statistical analyses using two-way ANOVA with Fisher’s LSD and outlier removal using the ROUT method, Q = 1%.
Wisniewski, K. E., Zhong, N. & Philippart, M. Pheno/genotypic correlations of neuronal ceroid lipofuscinoses. Neurology 57, 576–581 (2001).
Mole, S. E., Williams, R. E. & Goebel, H. H. Correlations between genotype, ultrastructural morphology and clinical phenotype in the neuronal ceroid lipofuscinoses. Neurogenetics 6, 107–126. https://doi.org/10.1007/s10048-005-0218-3 (2005).
Johnson, T. B. et al. Therapeutic landscape for Batten disease: current treatments and future prospects. Nat. Rev. Neurol. 15, 161–178. https://doi.org/10.1038/s41582-019-0138-8 (2019).
Consortium, T. I. B. D. Isolation of a novel gene underlying Batten disease, CLN3. The International Batten Disease Consortium. Cell 82, 949–957. https://doi.org/10.1016/0092-8674(95)90274-0 (1995).
Mirza, M. et al. The CLN3 gene and protein: What we know. Mol. Genet. Genom. Med. https://doi.org/10.1002/mgg3.859 (2019).
Cain, J. T. et al. Gene therapy corrects brain and behavioral pathologies in CLN6-Batten disease. Mol. Ther. 27, 1836–1847. https://doi.org/10.1016/j.ymthe.2019.06.015 (2019).
Geary, R. S., Norris, D., Yu, R. & Bennett, C. F. Pharmacokinetics, biodistribution and cell uptake of antisense oligonucleotides. Adv. Drug Deliv. Rev. 87, 46–51. https://doi.org/10.1016/j.addr.2015.01.008 (2015).
Kim, J. et al. Patient-customized oligonucleotide therapy for a rare genetic disease. N. Engl. J. Med. 381, 1644–1652. https://doi.org/10.1056/NEJMoa1813279 (2019).
Geraets, R. D. et al. Moving towards effective therapeutic strategies for neuronal ceroid lipofuscinosis. Orphanet J. Rare Dis. 11, 40. https://doi.org/10.1186/s13023-016-0414-2 (2016).
Kurosaki, T., Popp, M. W. & Maquat, L. E. Quality and quantity control of gene expression by nonsense-mediated mRNA decay. Nat. Rev. Mol. Cell Biol. 20, 406–420. https://doi.org/10.1038/s41580-019-0126-2 (2019).
Bidou, L., Allamand, V., Rousset, J. P. & Namy, O. Sense from nonsense: therapies for premature stop codon diseases. Trends Mol. Med. 18, 679–688. https://doi.org/10.1016/j.molmed.2012.09.008 (2012).
Mort, M., Ivanov, D., Cooper, D. N. & Chuzhanova, N. A. A meta-analysis of nonsense mutations causing human genetic disease. Hum. Mutat. 29, 1037–1047. https://doi.org/10.1002/humu.20763 (2008).
Miller, J. N. & Pearce, D. A. Nonsense-mediated decay in genetic disease: Friend or foe?. Mutat. Res. Rev. Mutat. Res. 762, 52–64. https://doi.org/10.1016/j.mrrev.2014.05.001 (2014).
Keeling, K. M. Nonsense suppression as an approach to treat lysosomal storage diseases. Diseases. 4(4), 32 (2016).
Nagel-Wolfrum, K., Moller, F., Penner, I., Baasov, T. & Wolfrum, U. Targeting nonsense mutations in diseases with translational read-through-inducing drugs (TRIDs). BioDrugs 30, 49–74. https://doi.org/10.1007/s40259-016-0157-6 (2016).
Mitchison, H. M. et al. Targeted disruption of the Cln3 gene provides a mouse model for Batten disease. The Batten Mouse Model Consortium [corrected]. Neurobiol. Dis. 6, 321–334. https://doi.org/10.1006/nbdi.1999.0267 (1999).
Cotman, S. L. et al. Cln3 Δex7/8 knock-in mice with the common JNCL mutation exhibit progressive neurologic disease that begins before birth. Hum. Mol. Genet. 11, 2709–2721. https://doi.org/10.1093/hmg/11.22.2709 (2002).
Schulz, A., Kohlschütter, A., Mink, J., Simonati, A. & Williams, R. NCL diseases—clinical perspectives. Biochim. Biophys. Acta 1801–1806, 2013. https://doi.org/10.1016/j.bbadis.2013.04.008 (1832).
Jalanko, A. & Braulke, T. Neuronal ceroid lipofuscinoses. Biochim. Biophys. Acta BBA Mol. Cell Res. 1793, 697–709. https://doi.org/10.1016/j.bbamcr.2008.11.004 (2009).
Chan, C. H., Mitchison, H. M. & Pearce, D. A. Transcript and in silico analysis of CLN3 in juvenile neuronal ceroid lipofuscinosis and associated mouse models. Hum. Mol. Genet. 17, 3332–3339. https://doi.org/10.1093/hmg/ddn228 (2008).
Codlin, S. & Mole, S. E. S. pombe btn1, the orthologue of the Batten disease gene CLN3, is required for vacuole protein sorting of Cpy1p and Golgi exit of Vps10p. J. Cell. Sci. 122, 1163–1173. https://doi.org/10.1242/jcs.038323 (2009).
Mitchison, H. M. et al. Structure of the CLN3 gene and predicted structure, location and function of CLN3 protein. Neuropediatrics 28, 12–14 (1997).
Sugimoto, K., Matsumoto, K., Kornberg, R. D., Reed, S. I. & Wittenberg, C. Dosage suppressors of the dominant G1 cyclin mutant CLN3-2: identification of a yeast gene encoding a putative RNA/ssDNA binding protein. Mol. Gen. Genet. MGG 248, 712–718. https://doi.org/10.1007/bf02191711 (1995).
Sleat, D. E., Sohar, I., Pullarkat, P. S., Lobel, P. & Pullarkat, R. K. Specific alterations in levels of mannose 6-phosphorylated glycoproteins in different neuronal ceroid lipofuscinoses. Biochem. J. 334(Pt 3), 547–551 (1998).
Mitchison, H. M. et al. Targeted disruption of the Cln3 gene provides a mouse model for Batten disease. Neurobiol. Dis. 6, 321–334. https://doi.org/10.1006/nbdi.1999.0267 (1999).
Schmidtke, C. et al. Lysosomal proteome analysis reveals that CLN3-defective cells have multiple enzyme deficiencies associated with changes in intracellular trafficking. J. Biol. Chem. 294, 9592–9604. https://doi.org/10.1074/jbc.RA119.008852 (2019).
Appu, A. P. et al. Cln3-mutations underlying juvenile neuronal ceroid lipofuscinosis cause significantly reduced levels of Palmitoyl-protein thioesterases-1 (Ppt1)-protein and Ppt1-enzyme activity in the lysosome. J. Inherit. Metab. Dis. 42, 944–954. https://doi.org/10.1002/jimd.12106 (2019).
Tyynela, J., Cooper, J. D., Khan, M. N., Shemilts, S. J. & Haltia, M. Hippocampal pathology in the human neuronal ceroid-lipofuscinoses: distinct patterns of storage deposition, neurodegeneration and glial activation. Brain Pathol. 14, 349–357 (2004).
Pontikis, C. C., Cotman, S. L., MacDonald, M. E. & Cooper, J. D. Thalamocortical neuron loss and localized astrocytosis in the Cln3Deltaex7/8 knock-in mouse model of Batten disease. Neurobiol. Dis. 20, 823–836. https://doi.org/10.1016/j.nbd.2005.05.018 (2005).
Palmieri, M. et al. mTORC1-independent TFEB activation via Akt inhibition promotes cellular clearance in neurodegenerative storage diseases. Nat. Commun. 8, 14338. https://doi.org/10.1038/ncomms14338 (2017).
Pontikis, C. C. et al. Late onset neurodegeneration in the Cln3-/- mouse model of juvenile neuronal ceroid lipofuscinosis is preceded by low level glial activation. Brain Res. 1023, 231–242. https://doi.org/10.1016/j.brainres.2004.07.030 (2004).
Kovacs, A. D. et al. Age-dependent therapeutic effect of memantine in a mouse model of juvenile Batten disease. Neuropharmacology 63, 769–775. https://doi.org/10.1016/j.neuropharm.2012.05.040 (2012).
Cialone, J. et al. Females experience a more severe disease course in Batten disease. J. Inherit. Metab. Dis. 35, 549–555. https://doi.org/10.1007/s10545-011-9421-6 (2012).
Kovacs, A. D. & Pearce, D. A. Finding the most appropriate mouse model of juvenile CLN3 (Batten) disease for therapeutic studies: the importance of genetic background and gender. Dis. Model Mech. 8, 351–361. https://doi.org/10.1242/dmm.018804 (2015).
Geraets, R. D. et al. A tailored mouse model of CLN2 disease: a nonsense mutant for testing personalized therapies. PLoS ONE 12, e0176526. https://doi.org/10.1371/journal.pone.0176526 (2017).
Sleat, D. E. et al. A mouse model of classical late-infantile neuronal ceroid lipofuscinosis based on targeted disruption of the CLN2 gene results in a loss of tripeptidyl-peptidase I activity and progressive neurodegeneration. J. Neurosci. 24, 9117–9126. https://doi.org/10.1523/JNEUROSCI.2729-04.2004 (2004).
Weimer, J. M. et al. Cerebellar defects in a mouse model of juvenile neuronal ceroid lipofuscinosis. Brain Res. 1266, 93–107. https://doi.org/10.1016/j.brainres.2009.02.009 (2009).
Weimer, J. M. et al. Visual deficits in a mouse model of Batten disease are the result of optic nerve degeneration and loss of dorsal lateral geniculate thalamic neurons. Neurobiol. Dis. 22, 284–293. https://doi.org/10.1016/j.nbd.2005.11.008 (2006).
Weimer, J. M., Kriscenski-Perry, E., Elshatory, Y. & Pearce, D. A. The neuronal ceroid lipofuscinoses: mutations in different proteins result in similar disease. NeuroMol. Med. 1, 111–124. https://doi.org/10.1385/nmm:1:2:111 (2002).
Gupta, P. et al. Disruption of PPT1 or PPT2 causes neuronal ceroid lipofuscinosis in knockout mice. Proc. Natl. Acad. Sci. USA 98, 13566–13571. https://doi.org/10.1073/pnas.251485198 (2001).
Miller, J. N., Kovács, A. D. & Pearce, D. A. The novel Cln 1(R151X) mouse model of infantile neuronal ceroid lipofuscinosis (INCL) for testing nonsense suppression therapy. Hum. Mol. Genet. 24, 185–196. https://doi.org/10.1093/hmg/ddu428 (2015).
Kopra, O. et al. A mouse model for Finnish variant late infantile neuronal ceroid lipofuscinosis, CLN5, reveals neuropathology associated with early aging. Hum. Mol. Genet. 13, 2893–2906. https://doi.org/10.1093/hmg/ddh312 (2004).
Kriscenski-Perry, E., Kovacs, A. D. & Pearce, D. A. Seizure susceptibility, phenotype, and resultant growth delay in the nclf and mnd mouse models of neuronal ceroid lipofuscinoses. J. Child Neurol. 28, 1137–1141. https://doi.org/10.1177/0883073813493667 (2013).
Morgan, J. P. et al. A murine model of variant late infantile ceroid lipofuscinosis recapitulates behavioral and pathological phenotypes of human disease. PLoS ONE 8, e78694. https://doi.org/10.1371/journal.pone.0078694 (2013).
Wheeler, R. B. et al. The gene mutated in variant late-infantile neuronal ceroid lipofuscinosis (CLN6) and in nclf mutant mice encodes a novel predicted transmembrane protein. Am. J. Hum. Genet. 70, 537–542. https://doi.org/10.1086/338708 (2002).
Brandenstein, L., Schweizer, M., Sedlacik, J., Fiehler, J. & Storch, S. Lysosomal dysfunction and impaired autophagy in a novel mouse model deficient for the lysosomal membrane protein Cln7. Hum. Mol. Genet. 25, 777–791. https://doi.org/10.1093/hmg/ddv615 (2016).
Damme, M. et al. Gene disruption of Mfsd8 in mice provides the first animal model for CLN7 disease. Neurobiol. Dis. 65, 12–24. https://doi.org/10.1016/j.nbd.2014.01.003 (2014).
Jankowiak, W. et al. Retinal degeneration in mice deficient in the lysosomal membrane protein CLN7. Investig. Ophthalmol. Vis. Sci. 57, 4989–4998. https://doi.org/10.1167/iovs.16-20158 (2016).
Bolivar, V. J., Scott Ganus, J. & Messer, A. The development of behavioral abnormalities in the motor neuron degeneration (mnd) mouse. Brain Res. 937, 74–82 (2002).
Kuronen, M. et al. Galactolipid deficiency in the early pathogenesis of neuronal ceroid lipofuscinosis model Cln8mnd: implications to delayed myelination and oligodendrocyte maturation. Neuropathol. Appl. Neurobiol. 38, 471–486. https://doi.org/10.1111/j.1365-2990.2011.01233.x (2012).
Kuronen, M., Lehesjoki, A. E., Jalanko, A., Cooper, J. D. & Kopra, O. Selective spatiotemporal patterns of glial activation and neuron loss in the sensory thalamocortical pathways of neuronal ceroid lipofuscinosis 8 mice. Neurobiol. Dis. 47, 444–457. https://doi.org/10.1016/j.nbd.2012.04.018 (2012).
Traina, G. et al. Lipofuscin accumulation and gene expression in different tissues of mnd mice. Mol. Neurobiol. 45, 247–257. https://doi.org/10.1007/s12035-012-8248-y (2012).
Koch, S. et al. Morphologic and functional correlates of synaptic pathology in the cathepsin D knockout mouse model of congenital neuronal ceroid lipofuscinosis. J. Neuropathol. Exp. Neurol. 70, 1089–1096. https://doi.org/10.1097/NEN.0b013e318238fc28 (2011).
Partanen, S. et al. Synaptic changes in the thalamocortical system of cathepsin D-deficient mice: a model of human congenital neuronal ceroid-lipofuscinosis. J. Neuropathol. Exp. Neurol. 67, 16–29. https://doi.org/10.1097/nen.0b013e31815f3899 (2008).
Arrant, A. E., Onyilo, V. C., Unger, D. E. & Roberson, E. D. Progranulin gene therapy improves lysosomal dysfunction and microglial pathology associated with frontotemporal dementia and neuronal ceroid lipofuscinosis. J. Neurosci. 38, 2341–2358. https://doi.org/10.1523/JNEUROSCI.3081-17.2018 (2018).
Smith, K. R. et al. Strikingly different clinicopathological phenotypes determined by progranulin-mutation dosage. Am. J. Hum. Genet. 90, 1102–1107. https://doi.org/10.1016/j.ajhg.2012.04.021 (2012).
Tanaka, Y., Chambers, J. K., Matsuwaki, T., Yamanouchi, K. & Nishihara, M. Possible involvement of lysosomal dysfunction in pathological changes of the brain in aged progranulin-deficient mice. Acta Neuropathol. Commun. 2, 78. https://doi.org/10.1186/s40478-014-0078-x (2014).
Schultheis, P. J. et al. Atp13a2-deficient mice exhibit neuronal ceroid lipofuscinosis, limited α-synuclein accumulation and age-dependent sensorimotor deficits. Hum. Mol. Genet. 22, 2067–2082. https://doi.org/10.1093/hmg/ddt057 (2013).
Tang, C.-H. et al. Murine cathepsin F deficiency causes neuronal lipofuscinosis and late-onset neurological disease. Mol. Cell. Biol. 26, 2309–2316. https://doi.org/10.1128/MCB.26.6.2309-2316.2006 (2006).
Macauley, S. L. et al. Cerebellar pathology and motor deficits in the palmitoyl protein thioesterase 1-deficient mouse. Exp. Neurol. 217, 124–135. https://doi.org/10.1016/j.expneurol.2009.01.022 (2009).
Oswald, M. J., Palmer, D. N., Kay, G. W., Barwell, K. J. & Cooper, J. D. Location and connectivity determine GABAergic interneuron survival in the brains of South Hampshire sheep with CLN6 neuronal ceroid lipofuscinosis. Neurobiol. Dis. 32, 50–65. https://doi.org/10.1016/j.nbd.2008.06.004 (2008).
Zetoune, A. B. et al. Comparison of nonsense-mediated mRNA decay efficiency in various murine tissues. BMC Genet. 9, 83. https://doi.org/10.1186/1471-2156-9-83 (2008).
Thada, V., Miller, J. N., Kovacs, A. D. & Pearce, D. A. Tissue-specific variation in nonsense mutant transcript level and drug-induced read-through efficiency in the Cln 1(R151X) mouse model of INCL. J. Cell Mol. Med. 20, 381–385. https://doi.org/10.1111/jcmm.12744 (2016).
Kovács, A. D. & Pearce, D. A. Finding the most appropriate mouse model of juvenile CLN3 (Batten) disease for therapeutic studies: the importance of genetic background and gender. Dis. Models Mech. 8, 351. https://doi.org/10.1242/dmm.018804 (2015).
Livak, K. J. & Schmittgen, T. D. Analysis of relative gene expression data using real-time quantitative PCR and the 2(-Delta Delta C(T)) method. Methods 25, 402–408. https://doi.org/10.1006/meth.2001.1262 (2001).
Poppens, M. J. et al. Tracking sex-dependent differences in a mouse model of CLN6-Batten disease. Orphanet J. Rare Dis. 14, 19. https://doi.org/10.1186/s13023-019-0994-8 (2019).
This work received support from the Sanford Research Imaging Core within the Sanford Research Center for Pediatric Research (NIH P20GM103620).
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Langin, L., Johnson, T.B., Kovács, A.D. et al. A tailored Cln3Q352X mouse model for testing therapeutic interventions in CLN3 Batten disease. Sci Rep 10, 10591 (2020). https://doi.org/10.1038/s41598-020-67478-5
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