Sphingolipids, lipids with a common sphingoid base (also termed long chain base) backbone, play essential cellular structural and signaling functions. Alterations of sphingolipid levels have been implicated in many diseases, including neurodegenerative disorders. However, it remains largely unclear whether sphingolipid changes in these diseases are pathological events or homeostatic responses. Furthermore, how changes in sphingolipid homeostasis shape the progression of aging and neurodegeneration remains to be clarified. We identified two mouse strains, flincher (fln) and toppler (to), with spontaneous recessive mutations that cause cerebellar ataxia and Purkinje cell degeneration. Positional cloning demonstrated that these mutations reside in the Lass1 gene. Lass1 encodes (dihydro)ceramide synthase 1 (CerS1), which is highly expressed in neurons. Both fln and to mutations caused complete loss of CerS1 catalytic activity, which resulted in a reduction in sphingolipid biosynthesis in the brain and dramatic changes in steady-state levels of sphingolipids and sphingoid bases. In addition to Purkinje cell death, deficiency of CerS1 function also induced accumulation of lipofuscin with ubiquitylated proteins in many brain regions. Our results demonstrate clearly that ceramide biosynthesis deficiency can cause neurodegeneration and suggest a novel mechanism of lipofuscin formation, a common phenomenon that occurs during normal aging and in some neurodegenerative diseases.
Lipids play many essential cellular roles as structural components of biological membranes or signaling molecules. Alterations of lipids have been observed in the brains of patients with neurodegenerative diseases. However, whether these changes can cause neurodegeneration or otherwise influence the pathology of these diseases is unclear. We identified mouse mutations in a gene encoding a neuronally expressed enzyme that generates ceramide, the basic structural component of many lipids known as sphingolipids. These mutations result in progressive ataxia and loss of cerebellar Purkinje cells. In addition, many neurons in these mutant mice harbor lipofuscin, a storage material containing both membranes and proteins, that is present in aging brains and in brains of patients with neurodegenerative disorders, suggesting that both membrane and protein homeostasis are impaired in mutant neurons. This study directly demonstrates that disruption of sphingolipid biosynthesis can lead to selective neuron death and the abnormal accumulation of lipofuscin, and it underscores the need for further study of the roles of lipids in neurodegenerative disorders.
Citation: Zhao L, Spassieva SD, Jucius TJ, Shultz LD, Shick HE, et al. (2011) A Deficiency of Ceramide Biosynthesis Causes Cerebellar Purkinje Cell Neurodegeneration and Lipofuscin Accumulation. PLoS Genet 7(5): e1002063. doi:10.1371/journal.pgen.1002063
Editor: Harry T. Orr, University of Minnesota, United States of America
Received: January 24, 2011; Accepted: March 17, 2011; Published: May 19, 2011
Copyright: © 2011 Zhao et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: Services used in this study were supported by CORE Grant CA34196 (The Jackson Laboratory). This work was also supported, in part, by Award Number I01BX000156 from the Biomedical Laboratory Research and Development Service of the VA Office of Research and Development (to LMO) and NIH/NIA R01 AG016583 (to LMO). LC-MS/MS analysis of sphingolipids was supported by NIH/NCRR SC COBRE Grant P20 RR017677. SLA is an investigator of the Howard Hughes Medical Institute. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
A hallmark of aging and many neurodegenerative disorders is the neuronal accumulation of storage materials. These deposits include lipofuscin that contain undigested membranes and defective proteins , and/or membrane-free aggregates of misfolded proteins . While the pathological roles of these accrued substances are unclear and may vary between diseases, their sequestration may protect neurons from those components that are otherwise highly toxic in soluble forms . However, evidence also suggests that insoluble storage materials are inherently toxic, and in some circumstances these materials may lead to the inhibition of proteasomal and lysosomal functions, which in turn accelerates their further deposition .
In addition to the accumulation of storage materials and impaired protein degradation capacity, changes in cellular homeostasis, including alterations in both simple and complex sphingolipid composition, also occur in the brains of patients with neurodegenerative diseases and in the aging brain , . These highly diverse lipids play important structural and signaling functions in the cell, and mediate cell-cell interaction , . Increases in levels of specific species of ceramide, the simplest sphingolipid, have been found in the brains of Alzheimer's disease (AD) patients and a mouse model of AD, and correlate with disease severity , , . Similarly, long-chain and very long-chain ceramide species are increased in the brains of HIV-associated dementia patients . Changes in several sphingolipid classes have been observed in the brains of patients with progressive epilepsy with mental retardation (EPMR), a form of neuronal ceroid lipofuscinosis (CLN8) . Furthermore, sphingolipids have been implicated in Parkinson's disease (PD) and Huntington's disease (HD) . For example, glucocerebrosidase mutations have been suggested to be risk factors for PD and other Lewy body disorders . Fibroblasts of HD patients and the brain of HD animal models exhibit reduced GM1 ganglioside levels . Lastly, changes in sphingolipids have also been associated with metabolic diseases that are caused by mutations of proteins involved in sphingolipid degradation. Storage of sphingolipids in these diseases results in global impairment of lysosomal function . This in turn blocks lysosomal degradation of defective proteins and organelles.
While we are beginning to understand the molecular pathology of sphingolipid-related and other lysosomal storage diseases, the roles of sphingolipid metabolism in the progression of aging and neurodegeneration are still not clear. It was reported that disruption of the Lass2 gene that encodes ceramide synthase 2 (CerS2), caused myelin degeneration, consistent with the restricted expression of this gene within the brain to oligodendrocytes, and secondary loss of cerebellar granule cells . This finding demonstrates that reduction of sphingolipid levels is indeed pathogenic in the brain, at least in oligodendrocytes. Here we report that deficiency of Lass 1 that encodes CerS1, a ceramide synthase that is predominantly expressed in neurons , , causes progressive Purkinje cell loss in mice. We also show that CerS1 plays a key role in ceramide biosynthesis in the brain, and loss of this protein dramatically impacts many aspects of sphingolipid homeostasis. Lastly, we find that loss of CerS1 leads to accumulation of lipofuscin that are associated with ubiquitylated proteins in many regions of the brain, suggesting that ceramide biosynthesis is critical for protein and organelle homeostasis. These data demonstrate that lipid biosynthesis defects in neurons can directly cause cell death. Furthermore, our results establish a causal link between lipid biosynthesis deficiencies and lipofuscin accumulation, and may provide a common mechanism for deposition of lipofuscin in aging and neurodegenerative diseases.
Cerebellar Purkinje cell defects in the flincher mutant brain
The flincher (fln) mutation arose spontaneously in a colony of NOD.CB17-Prkdcscid/SzJ mice at The Jackson Laboratory. Mice homozygous for the fln mutation were hyperactive and generally smaller in body size beginning at postnatal day seven. By three weeks of age, the size difference between mutant mice and their littermates was very obvious. Although mutant mice continued to gain weight until reaching maturity, adult mutant mice progressively lost weight, like other ataxic mice. However, the lifespan of mutant mice was comparable to that of their wild type or heterozygous littermates despite their weight loss and severe ataxia.
Flincher mutant mice displayed cerebellar ataxia beginning at three weeks, which was concomitant with degeneration of cerebellar Purkinje cells (Video S1, Figure 1A and data not shown). Neuron loss was progressive, and many Purkinje cells had degenerated in mutant mice by four months of age (Figure 1B–1D). Although the soma of Purkinje cells appeared normal in the mutant mice prior to three weeks of age, at postnatal day twelve (P12), Purkinje cell dendritic arbors were shorter than those in the wild type cerebellum (Figure 1E–1F). This reduction of dendritic arbor size was more pronounced by P17 (Figure 1G–1H). In addition, the reduced density of calbindin immunostaining in the molecular layer at P17 suggested that the complexity of higher order branches of mutant Purkinje cell dendritic arbors may also be reduced compared to that of wild type dendrites.
Figure 1. Progressive cerebellar Purkinje cell degeneration and abnormalities of Purkinje dendritic arbors in fln/fln mice.
(A–D) Calbindin D-28 immunostained sagittal sections of cerebella from three-week-old (B), four-week-old (B) and four-month-old fln/fln (C), and four-month-old wild type (+/+, D) mice. Sections were counterstained with hematoxylin. Cerebellar lobules are indicated by Roman numerals. (E–H) Purkinje cells immunostained with calbindin D-28 from wild type (E, G) and fln/fln (F, H) mice at P12 (E, F) and P17 (G, H). Scale bars: 1 mm (A–D); 50 µm (E–H).doi:10.1371/journal.pgen.1002063.g001
The flincher mutation disrupts the Lass1 gene
To identify the molecular defect in fln mutant mice, we crossed fln/fln and BALB/cByJ mice, and performed genome scans on F2 mice using sequence tagged site (STS) markers. This analysis localized the fln mutation to Chromosome 8. Fine mapping using these F2 mice and additional F2 mice from a fln×CAST/EiJ cross narrowed the fln mutation to a 0.04 cM (0.8 Mb) region between two single nucleotide polymorphisms (SNPs), D8SlacAT1 and rs6348000 (two recombinants/1984 F2 mice), containing 34 known protein-encoding genes (Figure 2A, Figure S1 and Figure S2A). To further define the mutant locus, transgenic mice carrying bacteria artificial chromosomes (BACs) containing genes from the fln critical interval were generated and crossed with mutant mice (Figure S2A). Among the three BACs used to make transgenic mice, only BAC RP23-349E13 was able to complement the fln mutant phenotype (Figure S2B–S2C). BAC RP23-349E13 contains nine known genes (Figure 2B) and the expression of one of these genes, Lass1, was greatly reduced in fln/fln brains (Figure 2C, left panels). Sequencing of Lass1 RT-PCR products revealed a single nucleotide deletion in exon 5, which results in a frameshift mutation that likely leads to nonsense-mediated decay of the Lass1 transcript in fln mutant brains (Figure 2D, left panels).
Figure 2. Genome mapping and identification of the flincher and toppler mutations.
(A) The critical mapping interval of the fln mutation is between D8SlacAT1 and rs6348000. (B) The genes encoded in BAC RP23-349E13 that was used to construct the fln-rescuing BAC transgenic line. (C) Northern blot analyses of fln/fln and to/to brain mRNA hybridized with probes to Lass1 and Gdf1. Blots were re-hybridized with a Gapdh probe as a loading control. (D) Sequence chromatograms of wild type (+/+), fln/fln and to/to Lass1 cDNA reveal a single nucleotide deletion (underlined in the wild type chromatogram) in fln/fln mice and a missense mutation (underlined) in to/to mice. (E–F) Calbindin D-28 immunohistochemistry of cerebella from 8-week-old fln/fln (E) and fln/fln; Tg(NSE-Lass1) (F) mice.doi:10.1371/journal.pgen.1002063.g002
Lass1 is transcribed as a part of an unusual bicistronic transcript that also encodes growth differentiation factor-1 (GDF1), a member of the TGF-ß family . Thus, as expected, Gdf1 expression is also reduced in fln mutant brains (Figure 2C, left panels). To determine if the fln phenotype is a result of loss of Lass1 or of decreased Gdf1 function, we performed cDNA transgenic complementation experiments. Transgenic mice expressing the Lass1 cDNA under the control of the neuron-specific enolase (NSE) promoter were generated and mated with fln mutant mice to generate fln/fln mice carrying the Lass1 transgene. These mice did not develop ataxia nor did they have Purkinje cell degeneration, demonstrating that expression of Lass1 in neurons is sufficient to rescue fln-mediated Purkinje cell degeneration (Figure 2E–2F and data not shown). Therefore, loss of Lass1, not Gdf1, function underlies the neuropathology observed in fln mutant mice.
Toppler (to) is a point mutation in the Lass1 gene
Toppler (to), a spontaneous recessive mutation causing Purkinje cell degeneration beginning around three weeks after birth, was also mapped to the middle of Chromosome 8 . Postnatal Purkinje cells in to mutant cerebella also display higher order dendritic branching pattern abnormalities. Based on the striking phenotypic similarity, we proposed that to and fln mutations were allelic and performed complementation tests. Fln/+; to/+ compound heterozygous mice exhibited progressive ataxia beginning at three weeks of age (data not shown). These mice also had Purkinje cell degeneration that was indistinguishable from that was observed in mice homozygous for either the to or the fln mutation (data not shown), indicating that the to mutation also likely disrupts the Lass1 gene. This inference was confirmed by the rescue of the to mutant phenotype by the Lass1 cDNA transgene (Figure S3A–S3B). Although the RNA expression level of the bicistronic Lass1-Gdf1 transcript was not affected by the to mutation (Figure 2C, right panels), sequencing of Lass1 RT-PCR products from toppler mutants revealed a missense point mutation in exon 5 resulting in the change of residue Ala266 to Asp (Figure 2D, right panel, and Figure S4B). These results confirmed that the Lass1 gene underlies the pathological changes in both fln and to mutant mice.
The fln and to mutations disrupt ceramide synthase 1 enzymatic activity
The Lass1 gene encodes the (dihydro)ceramide synthase CerS1, one of the six (dihydro)ceramide synthases (CerS1–CerS6) in mammals, encoded by Lass1 to Lass6, respectively . In the de novo pathway of ceramide biosynthesis, these enzymes catalyze the condensation of fatty acyl-CoA and dihydrosphingosine (dhS, also known as sphinganine) to produce dihydroceramide (Figure 3A). Dihydroceramide, in turn, is desaturated on the dhS backbone by dihydroceramide desaturase to form ceramide, which is the basic building block for complex sphingolipids. In vitro overexpression studies demonstrated that each of the six mammalian ceramide synthases has different fatty acyl-CoA substrate specificity and saturated C18:0 fatty acyl-CoA is the preferred substrate for CerS1 –. These studies also demonstrated that CerS1 could also use C16:0 and C20:0 fatty acid-CoA, albeit inefficiently, but not the unsaturated C18:1 fatty acyl-CoA that contains a Δ9 cis double bond .
Figure 3. The fln and to mutations impair ceramide synthase activity of CerS1.
(A) Schematic diagram of mammalian ceramide biosynthesis. (B–C) Ceramide synthase activities of brain microsomes from 12- to 13-day-old wild type (+/+, open bars; n = 5) and fln/fln mice (filled bars; n = 6). CerS activities for C18 fatty acyl-CoA (B) and C16 fatty acyl-CoA (C) are shown as mean ± SD. (D) In vitro C18 ceramide synthase activities of wild type and mutant CerS1 proteins. Full-length wild type CerS1 (CerS1wt), or CerS1H269trunc (Lass1fln) or CerS1A266D (Lass1to) were expressed in COS7 cells. Values are mean ± SD from three independent experiments. No significant difference of C18 ceramide synthase activity was observed between CerS1H269trunc and CerS1A266D. **: p≤0.01.doi:10.1371/journal.pgen.1002063.g003
Similar in vitro assays suggested that C18:0 fatty acyl-CoA can also serve as a substrate for CerS5, a CerS with broader substrate specificity . However, CerS5 is expressed at a lower level than that of CerS1 in the mouse brain . Together these data suggested that the reduction of CerS1 function in the mouse brain would significantly decrease the activities of ceramide synthases that utilize C18 fatty acyl-CoA. To test this hypothesis, we analyzed ceramide synthase activity with three fatty acyl-CoA substrates, including C18:0 fatty acyl-CoA, in microsomes prepared from wild type and mutant brain homogenates. The activity for C18 fatty acyl-CoA was reduced drastically in fln/fln brain microsomes, indicating that CerS1 is the major CerS in the brain using C18 fatty acyl-CoA (Figure 3B). No difference in ceramide synthase activity for C16 or C24 fatty acyl-CoA was observed between wild type and fln mutant brain microsomes, confirming the high specificity of CerS1 for C18 fatty acyl-CoA, and suggesting that the activities of other ceramide synthase isoenzymes present in the brain were not affected by the severely reduced CerS1 activity (Figure 3C and data not shown).
CerS1 is a multiple transmembrane domain protein and shares a conserved TRAM-LAG1-CLN8 (TLC) domain with other CerSs. The fln and to mutations reside between the last two predicted transmembrane domains. This region is within the TLC domain but outside of the LAG1 motif that was previously shown to be indispensible for the catalytic activity (Figure S4A) . Mice homozygous for either mutation have very similar phenotypes, suggesting that the Ala266Asp to mutation may also result in a dramatic loss of CerS1 function. To test this possibility, plasmids encoding wild type and mutant CerS1 proteins, each with an N- terminal FLAG epitope, were transfected into COS7 cells. Microsomes prepared from transfected cells were assayed for CerS activity using C18 fatty acyl-CoA as a substrate, and the crude enzymatic activity was normalized to the levels of FLAG-tagged CerS1. Both fln and to mutations impart almost complete loss of CerS1 catalytic activity, demonstrating that the carboxyl end of the TLC domain, and residue Ala266 in particular, are indispensible for CerS1 function (Figure 3D).
To investigate the effect of CerS1-deficiency on sphingolipid homeostasis in the brain, total lipids were extracted from wild type and fln mouse brains, and subjected to liquid chromatography coupled mass spectrometry (LC-MS). The total amount of ceramide was decreased by approximately 50%, confirming that CerS1 is a major CerS in the brain (Figure 4A). In line with the previous report on the preference of CerS1 for C18:0 fatty acyl-CoA, C18:0 ceramide was reduced approximately two fold in the mutant samples (Figure 4B). Although previous in vitro data demonstrated that unsaturated C18:1 fatty acyl-CoA was not utilized by CerS1 , the level of C18:1 ceramide was decreased more than five fold in the fln mutant brain suggesting that either CerS1 can utilize C18:1 fatty acyl-CoA in vivo, or the C18:1 side chain is formed by fatty acyl chain desaturation after ceramide biosynthesis (Figure 4C). Our results also confirm that C18 ceramide species are the dominant ceramide species in the mouse brain. Ceramide is the basic building block of complex sphingolipids, such as sphingomyelin and glycosphingolipids. In agreement with the reduced levels of C18 ceramide species, the amount of complex sphingolipids with C18 fatty-acyl groups was also reduced in the fln/fln brain (Figure S5A and data not shown).
Figure 4. Alterations of sphingolipid homeostasis in fln mutant brains.
Brain sphingolipid levels for selected sphingolipid species in 12- to 13-day-old wild type (+/+, open bars; n = 6) and fln/fln mice (filled bars; n = 5) were measured by mass spectrometry and normalized to protein concentration. Total ceramide (A), and C18:0 (B), C18:1 (C), and C16:0 (D) ceramide species are shown. Sphingosine (E), dihydrosphingosine (F), sphingosine-1-phosphate (G), dihydrosphingosine-1-phosphate (H) levels are also shown. All values are mean ± SD. **: p≤0.01.doi:10.1371/journal.pgen.1002063.g004
Contrary to the reduction of C18 sphingolipids observed in the fln mutant brain, the amounts of other long-chain sphingolipids, i.e. sphingolipids with fatty acyl chain length moiety C14 and C16, were increased significantly, suggesting a compensatory mechanism (Figure 4D, Figure S5 and data not shown). This compensation was not likely due to an upregulation of CerS5 or CerS6 that utilize C14 and C16 fatty acyl-CoA for ceramide biosynthesis, given that we did not observe an increased ceramide synthase activity with C16 fatty acid CoA in fln/fln brain microsomes (Figure 3C). Rather, increased C14 and C16 sphingolipid levels were most likely the result of excessive substrate availability for CerS5 and CerS6. The excessive substrate availability for CerS5 may also underlie the similar levels of C18 dihydroceramide observed in wild type and fln/fln brains (Figure S5C).
Sphingolipids undergo constant synthesis and degradation. Ceramide can be generated by degradation of complex sphingolipids, and be degraded further by ceramidases to release the sphingoid base, sphingosine. Sphingosine, in turn, can be recycled and used as the sphingoid substrate in the salvage pathway of ceramide biosynthesis, which is also catalyzed by CerSs (Figure 3A). Thus, loss of CerS1 function could result in accumulation of sphingosine, and dhS, the sphingoid substrate of de novo ceramide biosynthesis. Indeed, LC-MS analyses of fln/fln brains revealed a 2–4 fold increase in sphingosine and a greater than 10 fold increase in dhS (Figure 4E–4F). The phosphorylated metabolites of sphingosine and dhS, sphingosine-1-phosphate (S1P) and dhS-1-phosphate (dhS1P) were also significantly increased in mutant brains (Figure 4G–4H). However, the accumulation of dhS and dhS1P was much more pronounced than that of sphingosine and S1P, suggesting that the de novo ceramide biosynthesis pathway is the dominant pathway for ceramide biosynthesis in the brain.
Lipofuscin accumulates in CerS1 mutant brains
In normal aging brains and under some pathological conditions, undigested storage materials may accumulate in neurons to form autofluorecent deposits, termed lipofuscin. Based on the ultrastructure of lipofuscin, it has been suggested that lipofuscin production is a result of impaired autophagy of organelles, especially mitochondria . Consistent with this hypothesis, mutations of several lysosomal proteins have been linked to the neuronal ceroid lipofuscinoses (CLNs), a group of infantile- to juvenile-onset neurodegenerative diseases that are characterized by abnormal lipofuscin accumulation . However, the recent identification of two CLN proteins, CLN6 and CLN8, as polytopic membrane proteins on the endoplasmic reticulum suggests that non-lysosomal mechanisms may underlie lipofuscin accumulation in these diseases –. Although CLN8 does not show detectable ceramide synthase activity, ceramide profile changes have been observed in the brains of CLN8 patients . In addition, overexpression of CLN8 or CerSs suppressed the growth phenotype of fibroblasts from patients with CLN9, the causal gene of which has yet to be identified . These results indicate that defects in ceramide homeostasis may contribute to accumulation of lipofuscin.
To directly test whether a deficiency of ceramide biosynthesis can induce lipofuscin accumulation, we examined adult fln and to mutant brains. Although autofluorescent deposits were observed sporadically in neurons of four-month-old wild type mice, deposits were widespread in many brain regions in mutant mice, with the highest abundance in deep cerebellar nuclei, pons, medulla, anterior olfactory nuclei, layer IV to layer VI of the cerebral cortex, and the CA3 region of the hippocampus (data not shown). A similar pattern of deposits was observed in sections of mutant brains that were stained with Luxol fast blue, a compound that stains myelin and lipofuscin (Figure 5A–5B). To ascertain that these observed deposits are indeed lipofuscin, we examined their fine structure. Electron microscopy revealed the presence of many vacuoles and electron dense structures in the cytoplasm of mutant neurons (Figure 5C). Higher magnification revealed membranes and vacuoles within these dense structures, as typically seen in neuronal lipofuscin (Figure 5D).
Figure 5. Lipofuscin and ubquitylated protein accumulation in CerS1-deficient neurons.
(A–B) Sections of cerebella from four-month-old wild type (+/+, A) and fln/fln (B) mice were stained with Luxol Fast Blue. Images are converted to gray-scale for clear visualization of punctate staining. Images of the hippocampal CA3 region are shown. (C–D) Electron micrographs showing electron-dense deposits in fln/fln neurons at five months of age. An overview of a hippocampal neuron (C) showing vacuoles (arrowheads) and electron-dense deposits (arrows), and a lipofuscin structure from a cortical neuron (D) showing internal membrane structures (arrows) and vacuoles (arrowheads). (E–H) Ubiquitin immunohistochemistry of the hippocampal CA3 region from 4-month-old wild type (+/+, E, F) and fln/fln (G, H) mice. Details are shown in higher magnification (F, H). Conspicuous ubiquitylated accumulations in an fln/fln neuron are marked with arrows (H). (I–N) Ubiquitylated proteins (Ub; I, L) and autofluorescent lipofuscin (lipo; J, M) in a hippocampal neuron (I–K) and a cortical neuron (L–N) of a four-month-old fln/fln mouse. Merged images (K, N) show the relative locations of the ubiquitin immunofluorescent stain and autofluorescence. (O–Q) Ubiquitin-positive inclusions in Purkinje cells of three-week old fln/fln mice. Sections were incubated with an antibody against ubiquitin (O) and calbindin D-28 (P). Merged images are shown (Q), with Hoescht dye counterstaining. Scale bars: 20 µm (A–B); 2 µm (C); 100 nm (D); 50 µm (E, G); 20 µm (F, H, I–N); 25 µm (O–Q).doi:10.1371/journal.pgen.1002063.g005
Lipofuscin often contains both lipids and ubiquitylated proteins . To test whether ubiquitylated proteins also accumulate in the lipofuscin in CerS1 mutant brains, we performed immunohistochemistry using an antibody against ubiquitin. Indeed, ubiquitin-positive deposits were observed in the same types of neurons harboring lipofuscin, including cerebral cortical neurons, hippocampal CA3 neurons, and neurons in deep cerebellar nuclei, pons, medulla and anterior olfactory nuclei (Figure 5E–5H, and data not shown). Although the autofluorescent deposits are visible across a wide spectrum of light, the intensity of their fluorescence is lower than that of the fluorescent molecule-conjugated secondary antibodies used for ubiquitin immunofluorescence, allowing simultaneous assessment of lipofuscin and ubiquitin-positive puncta. We found that ubiquitylated proteins and autofluorescent deposits were largely colocalized or closely associated (Figure 5I–5N). While lipofuscin accumulated in many neurons in the mutant brain, we did not observe overt death of neurons other than Purkinje cells, although we cannot rule out more subtle changes in the survival of mutant neurons. However, as evidenced by the hyperactivity of CerS1 mutant mice, it is likely that the function of additional neurons is impaired in these mice.
Although lipofuscin deposition was much more pronounced in brains of older mutant mice, we also observed weak autofluorescent deposits containing ubiquitin-positive puncta in the soma and swollen dendrites of a small number of Purkinje cells in 3-week old mutant, but not wild type, mice (Figure 5O–5Q and data not shown). This result suggests that CerS1-deficiency also causes accumulation of lipofuscin-like structures in at least some Purkinje cells.
Alterations of sphingolipids have been observed in many neurodegenerative disorders. However, the contribution of these changes to disease pathogenesis is not clear . We have uncovered two spontaneous mutants with progressive degeneration of cerebellar Purkinje neurons and widespread lipofuscin accumulation. By positional cloning, we identified the mutations as alleles of the Lass1 gene, which encodes ceramide synthase 1 (CerS1), one of the six ceramide synthases in mammals. Our data demonstrate that deficiency of CerS1/LASS1 leads to dramatic alterations in the levels of sphingolipids in the brain, degeneration of cerebellar Purkinje neurons, and widespread lipofuscin accumulation.
CerS1 is specifically expressed in neurons in the brain and has been shown to produce C18:0 ceramide species in vitro or in cultured cells , , –. In the brain of Lass1 mutant mice, C18 sphingolipid species were significantly reduced, confirming the role of CerS1 in C18 ceramide biosynthesis in vivo. Loss of CerS1 also led to a decrease in total ceramide, in agreement with C18 ceramide as a major ceramide in the adult brain . However these sphingolipid decreases were accompanied by an increase in the steady state levels of C14 and C16 sphingolipid species. In addition, sphingoid bases and their phosphorylated metabolites were drastically increased in the mutant brain.
In contrast to previous reports suggesting that ceramide is proapoptotic in vitro and can mediate both stress-induced intrinsic and death receptor-mediated extrinsic apoptosis , , our data suggest that reduction of ceramide or complex sphingolipids results in progressive neuron death, particularly Purkinje cell loss. Intracerebroventricular administration of global ceramide inhibitors has been reported to cause acute neurodegeneration . Contrary to in vitro data, this finding, together with our results, demonstrate that decreases in ceramide synthesis can induce neuron death in vivo. Sphingolipid homeostasis is critically balanced in the cell under normal conditions, and thus either increases or decreases of ceramide could be detrimental to the cell. Alternatively, ceramide species with different fatty acyl chains may play distinct physiological roles. For example, loss of one of the two worm ceramide synthases, which produce different ceramide species, resulted in opposite outcomes in C. elegans under hypoxic conditions . Perhaps C18 ceramide, or some of its derived sphingolipids such as C18-sphingomyelin or C18-cerebrosides, act in a prosurvival fashion in neurons, whereas an increase in other ceramide species, such as C16 ceramide, may be apoptotic . Lastly, Purkinje neuron loss may be due to an increase in the sphingoid bases that normally serve as substrates for CerS1. Sphingoid bases, particularly their phosphorylated metabolites, are potent signaling molecules and have been proposed to regulate many signal transduction pathways . Thus, elevation of these molecules, particularly dhS and dhS1P, which are increased over ten fold in the CerS1-deficient brain, may impair normal functions of sphingolipid signaling, leading to Purkinje cell death.
Consistent with previous reports demonstrating that sphingolipid biosynthesis is crucial for dendritic development in cultured Purkinje or hippocampal neurons , , we observed shortened dendritic arbors and decreased density of calbindin immunostaining in the molecular layer in CerS1-deficient cerebella suggesting that dendritic development of mutant Purkinje cells was abnormal. The role of sphingolipids in dendritic development is not clear, but may involve sphingolipid-rich lipid rafts, which are implicated in activity-dependent dendritic development and maintenance of dendritic spines in in vitro experiments , . Dendritic dysfunction or morphological anomalies are often associated with neurodegeneration . While we cannot rule out a secondary cause for abnormalities in Purkinje cell dendrites in CerS1 mutant mice, it is possible that defects in dendritic development also contribute to death of these neurons.
In addition to Purkinje cell death, our data clearly demonstrate that deficiency of ceramide biosynthesis can cause the accumulation of lipofuscin, which is often observed in aging brains and in some neurodegenerative diseases. Lipofuscin is known to contain both lipids and proteins that may originate from membrane bound organelles such as mitochondria . Accumulation of lipofuscin has been linked to reduced lysosomal hydrolytic capacity, based on observations of lipofuscin deposition in mutants with deficiencies in lysosomal proteins , . Both increases and decreases in ceramide have been shown to induce autophagy, suggesting that the balance of sphingolipid homeostasis is important for autophagy and/or lysosomal functions , . Alternatively, conditions that increase the load on lysosomes beyond their capacity may also underlie lipofuscin formation. Given the importance of sphingolipids in protein targeting and as components of membranes, reduced sphingolipid levels may increase the demand on, and/or decrease the capacity of lysosomal function by affecting both lysosomal and non-lysosomal membrane dynamics, and targeting of membrane proteins. Increased load of defective membrane organelles and mislocalized membrane proteins could exceed lysosomal hydrolytic capacity of neurons, resulting in lipofuscin formation.
Previous reports suggest ceramide might also be important during aging . One of the yeast genes encoding ceramide synthases, LAG1 (longevity assurance gene 1), was identified in a screen for genes whose expression changed over yeast replicative cycles . Deletion of LAG1 was associated with an increase of replicative life span in yeast. However, a LASS1 variant exhibiting increased expression, when combined with specific HRAS1 and APOE haplotypes, was suggested to contribute to healthy aging and survival in a human population . This finding suggests that appropriately increased ceramide levels might be beneficial to some cells in aging animals. Inversely, given the specificity of Purkinje cell loss observed in CerS1-deficient mice, decreased ceramide levels appear more detrimental to neurons, and accelerate aging phenotypes, including lipofuscin accumulation. Thus our results demonstrate that in addition to neurodegeneration, alteration of ceramide levels can accelerate some aspects of aging. More research is needed to elucidate the role of ceramide and other sphingolipids in aging and neurodegeneration.
Materials and Methods
All experiments with mice have been approved by The Jackson Laboratory Animal Care and Use Committee according to relevant national and international guidelines.
DNA oligos and genotyping assays
Mouse strains and plasmids
The fln and to mutations were maintained on a NOD/SzJ background and a FVB/N background, respectively. Bacterial artificial chromosome (BAC) transgenic mouse lines were generated by injection of purified BAC DNA into C57BL/6J pronuclei and maintained on the same background. To generate Lass1 cDNA transgenic lines, Lass1 cDNA was amplified from a mouse cDNA library plasmid pME18-FL3-LASS1 (Open Biosystems) with primers LZO455 and LZO456, and inserted into pNSE-Ex4N1 at the BamHI and SpeI sites, downstream of the neuron-specific enolase 2 gene (Nse2) promoter. The plasmid pNSE-Ex4N1 is a modified version of pNSE-Ex4, which was described previously , with BamHI, NotI and SpeI sites on an adapter inserted into the HindIII site of pNSE-Ex4. A SalI fragment containing the Lass1 cDNA, the Nse2 promoter and an SV40 polyadenylation sequence was used for pronuclear microinjection. For expression of full-length wild type LASS1 protein in cultured mammalian cells, the Lass1 coding region was recovered from the pNSE-Ex4N1-LASS1 plasmid by restriction digestion with BamHI and EcoRI, and was inserted into pCMV-3Tag-1A (Stratagene), in frame with a 3xFLAG epitope. For expression of mutant LASS1 proteins, Lass1 fragments were amplified from poly A+ RNA isolated from fln/fln or to/to mutant brains, using primers LZO605 and LZO606. The FLAG epitope-tagged wild type LASS1 construct was cleaved with BsrGI to swap an internal fragment with the fragments containing the mutations.
Homozygous fln mice were crossed with BALB/cByJ mice, and F1 heterozygotes were intercrossed to generate F2 mice. Genome scans using polymorphic microsatellite markers were performed on DNA from ten affected and ten unaffected F2 mice. To fine map the mutation, 951 F2 mice were analyzed using polymorphic microsatellite markers and single nucleotide polymorphisms (SNPs). To further narrow the critical interval, fln/fln and CAST/EiJ were crossed, and F1 heterozygotes were intercrossed to generate F2 mice. 1033 F2 mice were analyzed.
Preparation of RNA and northern blot analyses
Total brain RNA preparation, poly-A+ RNA selection and northern blot analyses were performed as described . To generate northern blot probes, fragments of Lass1 and Gdf1 coding sequences were amplified with oligos LZO463 and LZO426, and oligos LZO445 and LZO446, respectively.
Histology and immunohistochemistry
Immunohistochemical studies were performed as described . Briefly, mice were intracardically perfused and brains were postfixed before dehydration and embedding in paraffin. After antigen retrieval in 0.01 M citrate buffer (pH 6), sections were incubated at 4°C overnight with mouse monoclonal antibody against calbindin D-28 (Sigma-Aldrich, 1:1000) or rabbit polyclonal antibody against ubiquitin (DAKO, 1:200) in phosphate-buffered saline with 0.03% Triton and 5% normal donkey serum. Colorimetric Calbindin D-28 immunohistochemistry was performed as described . Fluorescent detection was performed with Alexa Fluor-conjugated secondary antibodies (Invitrogen, 1:200). Autofluorescence was quenched by incubation with 0.01% Sudan Black in 70% ethanol, and some sections were counterstained with Hoescht 33258. To detect autofluorescent deposits, deparaffinated sections were mounted with Fluoromount-G (Southern Biotech) without incubation with Sudan Black.
For electron microscopy, mice were intracardically perfused with a mixture of 1.2% paraformaldehyde and 0.8% glutaraldehyde, and brains were postfixed and processed for transmission electron micrography using standard procedures .
Cell culture and transfection
COS7 cells were cultured in Dulbecco's Modified Eagle's Medium (Invitrogen) supplemented with 10% Fetal Bovine Serum (Hyclone). Transfections were performed using Lipofectamine 2000 (Invitrogen) according to the manufacturer's protocol. Medium was replaced with fresh medium 12 hours after the transfection, and cells were harvested 48 hours after transfection.
Microsomal preparation and in vitro ceramide synthase assays
For microsomal preparation from mouse brains, the tissue was homogenized in 20 mM HEPES buffer (pH 7.4, 2 mM KCL, 2 mM MgCl2, 250 mM sucrose) supplemented with protease inhibitors (Sigma) with a Tissue Tearor homogenizer (Biospec Products). For microsomal preparation from culture cells, harvested cells were lysed in 20 mM HEPES buffer (see above) with a 30-gauge syringe. Tissue homogenates or cell lysates were subjected to centrifugation at 1,000×g for 5 min at 4°C to remove unbroken tissue debris or intact cells and nuclei. The supernatants were subjected to centrifugation at 10,000×g for 10 min at 4°C to remove mitochondria. The supernatants were ultracentrifuged at 100,000×g for 1 h at 4°C to collect microsomes, which were re-suspended in HEPES buffer (see above), and protein concentrations were measured with the Bradford method (BioRad). For in vitro ceramide synthase assays, a 100 µL reaction mixture containing 15 µM C17 sphingosine (Avanti Polar Lipids) and 50 µM C16, C18 or C24 fatty acid CoA (Avanti Polar Lipids) in 25 mM potassium phosphate buffer (pH 7.4) was pre-warmed at 37°C for 5 min. The enzymatic reaction was initiated by adding microsomes (15 µg) to the reaction mixture, which was incubated at 37°C for 15 min, and the reaction was terminated by adding 2 mL extraction solvent (ethyl acetate/iso-propanol/water at 60/30/10 v/v/v), supplemented with d13/C16 ceramide and d13/C22 ceramide as internal standards for mass spectrometry analyses.
Lipid extraction and liquid chromatography/mass spectrometry (LC/MS) analyses of sphingolipids
Lipid extractions and LC/MS analyses were performed as described previously . Briefly, samples were fortified with internal standards. Lipids were extracted twice with 2 ml ethyl acetate/isopropanol/water (60/30/10 v/v) solvent system, dried under a stream of nitrogen, re-suspended into 150 µL 1 mM NH4COOH in 0.2% HCOOH in methanol, and analyzed by LC/MS. LC/MS analyses of sphingolipids were performed on a Thermo Finnigan TSQ 7000 triple quadrupole mass spectrometer, operating in a Multiple Reaction Monitoring positive ionization mode. Sphingolipid levels in the brain homogenates were normalized to protein concentration measured by the Bradford method.
Protein samples were separated on SDS gels (BioRad) and transferred to a nitrocellulose membrane (Amersham Biosciences) using standard techniques . FLAG-tagged proteins were detected using M2 mouse monoclonal antibody against FLAG (Sigma). Mouse monoclonal N+/K+-ATPase antibody (Abcam) was used as a loading control. Primary antibodies were detected with an appropriate secondary antibodies conjugated with horseradish peroxidase, and detected with ECL (Amersham Pharmacia).
In vitro ceramide synthase assays and mass spectrometry data were analyzed with Sigma Plot. Paired t-tests were performed.
Haplotypes of selected recombinants used to refine the critical interval of the fln mutation. F2 recombinants from NOD.CB17-Prkdcscid/J-fln×BALB/cJ and NOD.CB17-Prkdcscid/J-fln×CAST/EiJ crosses are shown with the number of recombinants with each haplotype indicated.
BAC rescue of the fln mutation. (A) The critical interval of the flincher mutation. The three BAC clones used in the BAC complementation experiments are shown. (B–C) Calbindin-D28 immunostaining of cerebellar sections from a seven-week-old fln/fln mouse and an age-matched fln/fln littermate carrying the BAC RP23-349E13 transgene. Scale bar: 1 mm (B–C).
A neuron-specific Lass1 cDNA transgene suppresses the toppler mutation. Calbindin D-28 immunohistochemistry of cerebellar sections from eight-week-old to/to (A) and to/to; Tg(NSE-Lass1) (B) mice. Scale bar: 1 mm.
The fln and the to mutations are in the conserved TLC domain. (A) Predicted secondary structure of the mouse CerS1. Transmembrane domains were predicted with the TMPred server (http://www.ch.embnet.org/software/TMPRED_form.html) and combined with topological data of yeast ceramide synthases . The to and the fln mutations are marked with arrowheads. The TLC domain is indicated in light green, and the LAG1 motif in the TLC domain is shaded in darker green. (B) Alignment of CerS1 orthologs using COBALT (http://www.ncbi.nlm.nih.gov/tools/cobalt/). Identical or similar residues across all species are colored red or orange, respectively. Residues conserved in vertebrates are indicated in yellow. Transmembrane domains were marked according to the mouse CerS1 sequence. Arrowheads denote the fln and the to mutations. Residues that are identical or conserved in mouse CerS1–CerS6 are marked with filled and open circles, respectively. Sequences used for analysis are NP_067090 (human), NP_619588 (mouse), NP_001037695 (rat), CAK11083 (Zebra fish), NP_727075 (Drosophila, fly), and NP493403 (C. elegans, worm).
Mass spectrometry data showing profound changes of sphingolipids in the fln mutant brain. Brain sphingolipid levels in 12- to 13-day-old wild type (+/+, open bars; n = 5) and fln/fln mouse brains (filled bars; n = 6) were measured by mass spectrometry and normalized to protein concentration. (A) Abundance of sphingomyelin with different fatty acyl chain moieties. (B) Abundance of ceramide with different fatty acyl chain moieties. Note that C16 and C18 ceramide species are shown in Figure 4, and are not included here. (C) Abundance of dihydroceramide with different fatty acyl chain moieties. All values are mean ± SD. *: p≤0.05; **: p≤0.01.
Primers used to construct plasmids or used for genotyping.
Mice homozygous for the fln mutation display severe cerebellar ataxia. A four-month old fln/fln and an age-matched wild type (+/+) littermate are shown.
We thank The Jackson Laboratory sequencing, histology, microinjection and imaging services for their contributions; Dr. R. Bronson for assistance with electron microscopy; L. Marquis and J. Cook for technical assistance; and Drs. R. Burgess and W. Frankel for comments on the manuscript. We also thank the Lipidomics core facility at MUSC for mass spectrometry.
Conceived and designed the experiments: LZ SDS SLA. Performed the experiments: LZ SDS TJJ. Analyzed the data: LZ SDS SLA. Contributed reagents/materials/analysis tools: LDS HES WBM. Wrote the paper: LZ SDS SLA. Oversaw experiments: YAH LMO SLA.
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