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Molecular and Cellular Biology, December 2005, p. 11113-11121, Vol. 25, No. 24
0270-7306/05/$08.00+0     doi:10.1128/MCB.25.24.11113-11121.2005
Copyright © 2005, American Society for Microbiology. All Rights Reserved.

Essential Role for Sphingosine Kinases in Neural and Vascular Development

Kiyomi Mizugishi,1 Tadashi Yamashita,1 Ana Olivera,2 Georgina F. Miller,3 Sarah Spiegel,4 and Richard L. Proia1*

Genetics of Development and Disease Branch, NIDDK,1 Molecular Immunology and Inflammation Branch, NIAMS,2 Division of Veterinary Resources, National Institutes of Health, Bethesda, Maryland 20892,3 Department of Biochemistry, Virginia Commonwealth University School of Medicine, Richmond, Virginia 232984

Received 8 August 2005/ Returned for modification 10 September 2005/ Accepted 1 October 2005


   ABSTRACT
Top
 Abstract
Introduction
 Materials and Methods
 Results
 Discussion
 References
 
Sphingosine-1-phosphate (S1P), an important sphingolipid metabolite, regulates diverse cellular processes, including cell survival, growth, and differentiation. Here we show that S1P signaling is critical for neural and vascular development. Sphingosine kinase-null mice exhibited a deficiency of S1P which severely disturbed neurogenesis, including neural tube closure, and angiogenesis and caused embryonic lethality. A dramatic increase in apoptosis and a decrease in mitosis were seen in the developing nervous system. S1P1 receptor-null mice also showed severe defects in neurogenesis, indicating that the mechanism by which S1P promotes neurogenesis is, in part, signaling from the S1P1 receptor. Thus, S1P joins a growing list of signaling molecules, such as vascular endothelial growth factor, which regulate the functionally intertwined pathways of angiogenesis and neurogenesis. Our findings also suggest that exploitation of this potent neuronal survival pathway could lead to the development of novel therapeutic approaches for neurological diseases.


   INTRODUCTION
Top
 Abstract
 Introduction
Materials and Methods
 Results
 Discussion
 References
 
Sphingosine-1-phosphate (S1P) is a signaling molecule that is crucial for the regulation of several diverse cellular events, including cell survival, growth, differentiation, motility, and calcium mobilization (29). Recently, numerous studies on S1P have demonstrated its importance in the development of the vascular system (1, 14, 16, 18), the heart (15), and immunity (2, 5, 21) by signaling through a family of G protein-coupled receptors designated S1P1 to S1P5. The S1P signaling pathway through S1P receptors induces activation of the protein kinase Akt, phosphatidylinositol 3-kinase, the small GTPase Rac, phospholipase C, and extracellular signal-regulated kinase, leading to cell survival and proliferation (11). In higher plants, S1P also plays an important role in calcium regulation and the control of guard cells (7).

Sphingosine kinase (SphK) is an enzyme that catalyzes the phosphorylation of sphingosine to form S1P. Two isoforms of mammalian SphK (SphK1 and SphK2) have been cloned and characterized (13, 17). Recent studies revealed that overexpression of SphK2 suppressed cell growth and also markedly enhanced apoptosis in cultured cells (12, 19), in sharp contrast to findings for SphK1, which generally promoted cell survival and growth (26, 27).

Recently, we generated SphK1 knockout mice to study the enzyme's physiological functions (3). The SphK1–/– mice were viable and fertile and lacked any obvious abnormalities, although total SphK activity was substantially, but not completely, reduced. These results raise the possibility that SphK1 and SphK2 might have redundant functions in mice and that SphK2 could compensate for a deficiency in SphK1 activity. To investigate the physiological functions of both isoforms, we generated SphK2 knockout mice, as well as SphK1/SphK2 double-knockout mice. Simultaneous deletion of both enzymes resulted in mice with undetectable levels of S1P. The studies on S1P-deficient mice described herein reveal a novel function for S1P signaling in neural development, in addition to its established role in vascular development.


   MATERIALS AND METHODS
Top
 Abstract
 Introduction
 Materials and Methods
Results
 Discussion
 References
 
Generation of SphK2 mutant mice. An 18.5-kb genomic DNA fragment of SphK2 was cloned from a 129/Sv library and characterized. As shown in Fig. 1A, mouse SphK2 consists of seven exons, with the coding region located in exons 3 to 7. A plasmid construct was created by replacing the region from the second half of exon 4 to the end of exon 7 with a LacZ-Neo cassette containing an internal ribosomal entry sequence. This targeting strategy should allow both disruption of the SphK2 allele and analysis of SphK2 expression in mice by creation of an SphK2-LacZ hybrid transcript driven by endogenous SphK2 promoter elements. The herpes simplex virus thymidine kinase gene was located outside of the homologous sequence to prevent random integration. Correctly targeted embryonic stem cell clones were injected into C57BL/6 blastocysts, producing chimeric mice. Highly chimeric males were mated to C57BL/6 females, and then the progenitors were intercrossed.


Figure 1
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  		FIG. 1. Targeted disruption of the SphK2 gene. (A) Schematic representation of the SphK2 targeting strategy. The structure of the SphK2 targeting vector is shown at the top, the mouse SphK2 locus in the middle, and the predicted structure of the homologous recombined locus, with the location of the Southern probe, at the bottom. P1 and P2 were used for RT-PCR. B, BamHI; Bg, BglII; N, NotI; S, SpeI; X, XhoI; pBS; pBluescript vector. (B) Southern blot analysis of SpeI-digested genomic tail DNA from mice generated by SphK2 heterozygous mating. The wild-type SphK2 locus yielded a 7.0-kb SpeI band. The disrupted SphK2 locus yielded a 10.9-kb SpeI band. (C) RT-PCR analysis of total RNA from adult tissues with primers P1 and P2. SphK2+/+ RNA yielded the predicted 195-bp amplification product. No amplification product was detected from SphK2–/– RNA. GAPDH, glyceraldehyde-3-phosphate dehydrogenase.

 
Genotyping of SphK1, SphK2, and S1P1 mutant mice. Genotyping for the S1P1 and SphK1 alleles was performed as previously described (3, 18). Genotyping for SphK2 alleles was done by Southern blot or PCR analysis. For Southern blot analysis, SpeI-digested DNA was probed with a radiolabeled 3' sequence that was located outside of the recombination site shown in Fig. 1A. For PCR analysis, genomic DNA was used as the template (40 cycles of 94°C for 30 s, 55°C for 30 s, and 72°C for 2 min) with primers P3 (5'-GCACCCAGTGTGAATCGAGC-3'), P4 (5'-TCTGGAGACGGGCTGCTTTA-3'), and P5 (5'-CGCTATCAGGACATAGCGTT-3'). Expected product sizes for the wild-type and targeted alleles were 680 and 310 bp, respectively.

RT-PCR. Total RNA was isolated with Trizol (Invitrogen). Total RNA (1 µg) was reverse transcribed with the SuperScript First-Strand Synthesis System for reverse transcription (RT)-PCR (Invitrogen) by following the manufacturer's instructions. PCR for SphK2 alleles was performed with primers P1 (5'-ACCACTTATGAGGAGAATCG-3') and P2 (5'-CACCACGTGGTCCATACAGC-3'). Glyceraldehyde-3-phosphate dehydrogenase was used to monitor RNA recovery. The primer pairs used for amplification of the glyceraldehyde-3-phosphate dehydrogenase gene were from Applied Biosystems. Each PCR cycle consisted of 30 s of denaturation at 94°C, 30 s of annealing at 55°C, and 2 min of extension at 72°C.

Measurement of SphK activity. SphK activity was measured essentially as described previously (25). Homogenates from embryos at embryonic day 11.5 (E11.5) (15 µg of protein in sphingosine kinase buffer containing 50 mM Tris [pH 7.5], 10% glycerol, 1 mM ß-mercaptoethanol, 1 mM EDTA, 1 mM sodium orthovanadate, 40 mM ß-glycerophosphate, 15 mM NaF, 10 µg/ml each leupeptin and aprotinin, 1 mM phenylmethylsulfonyl fluoride, and 0.5 mM 4-deoxypyridoxine) were incubated with 50 µM sphingosine (prepared either in mixed micelles with Triton X-100 or in bovine serum albumin [BSA] complexes without Triton X-100), 10 µCi of [{gamma}-32P]ATP (1 mM), and 10 mM MgCl2. Labeled lipids were extracted and resolved by thin-layer chromatography as described previously (25). Labeled S1P was quantified with a PhosphorImager.

Measurement of S1P levels. S1P levels in embryos at E11.5 were essentially measured as described previously (9, 13). Lipids from homogenates from embryos at E11.5 were extracted by adding 1 ml of 25 mM HCl-1 M NaCl, 1 ml of methanol, 1 ml of chloroform, and 100 µl of 3 N NaOH and phases separated. The aqueous phase containing S1P, devoid of sphingosine and the majority of phospholipids, was transferred to a siliconized glass tube. The organic phases were re-extracted with 1 ml of methanol-1 M NaCl (1:1, vol/vol) and the aqueous fractions combined. Mass levels of S1P in the pooled aqueous phases were determined exactly as described previously (13).

Measurement of sphingosine levels. Lipids from homogenates of embryos at E11.5 were extracted by adding 1 ml of 25 mM HCl-1 M NaCl, 1 ml of methanol, 1 ml of chloroform, and 100 µl of 3 N NaOH. After phase separation, the aqueous phase containing S1P was transferred to a siliconized glass tube and the organic phases were re-extracted with 1 ml of methanol-1 M NaCl (1:1, vol/vol). Aliquots of the lower organic phase containing sphingosine were dried under nitrogen and then resuspended in sphingosine kinase buffer with Triton X-100. Sphingosine converted to S1P was measured as described previously (9).

Histological analysis. Embryos were removed from the mother, fixed, and processed to be embedded in paraffin. Serial sections (5 µm) were made at 15- to 30-µm intervals and stained with hematoxylin and eosin (H&E). Immunostaining of vascular smooth muscle cells was performed with anti-smooth muscle {alpha}-actin antibody (Dako Cytomation). Paraffin sections were deparaffinized and rehydrated. Antigen retrieval was accompanied by 10-min incubation at 95°C in Target Retrieval Solution (Dako Cytomation). Endogenous peroxidase activity was quenched by incubation with 3% hydrogen peroxide in water for 5 min. Specimens were incubated with anti-smooth muscle {alpha}-actin for 1 h at room temperature. After washing with phosphate-buffered saline (PBS), the peroxidase reaction was visualized with diaminobenzidine-hydrogen peroxide. Mitotic cells were reacted with 1:100-diluted anti-phospho histone H3 antibody (Upstate) overnight at 4°C. After that, they were reacted with 1:1,000-diluted, peroxidase-conjugated goat anti-rabbit immunoglobulin G (Upstate) for 30 min at room temperature and then visualized with diaminobenzidine-hydrogen peroxide.

Whole-mount immunostaining. Embryos were fixed in 4% paraformaldehyde in PBS at 4°C overnight. They were then dehydrated through a methanol series and stored in 100% methanol at –20°C. The embryos were bleached in 5% hydrogen peroxide-methanol for 1 h at room temperature and rehydrated through a methanol series to PBS plus 0.1% Triton X-100 (PBST). They were incubated in a blocking solution (4% BSA in PBST) twice, for 1 h each time. The embryos were incubated with rat anti-mouse CD31 antibody (anti-PECAM-1; PharMingen) diluted 1:10 in 4% BSA in PBST at 4°C overnight. Embryos were washed with 4% BSA in PBST at 4°C and then incubated with 1:100-diluted, peroxidase-conjugated goat anti-rat immunoglobulin G (Jackson ImmunoResearch) in 4% BSA in PBST at 4°C overnight. Peroxidase reaction was visualized with diaminobenzidine-hydrogen peroxide.

Whole-mount X-Gal staining. Embryos were fixed in 2% formaldehyde-2% glutaraldehyde in PBS for 1 h. They were washed in PBS and then incubated in PBS containing 5 mM K3Fe(CN)6, 5 mM K4Fe(CN)6, 2 mM MgCl2, and 1 mg/ml 5-bromo-4-chloro-3-indolyl-ß-D-galactopyranoside (X-Gal) at 37°C for 2 h to 12 h. Reactions were stopped by rinsing embryos with PBS, followed by further fixation in 4% formaldehyde.

Whole-mount in situ hybridization. In situ hybridization was performed essentially as described previously (31). The cDNA fragment corresponding to the entire open reading frame and the fragment including part of the C terminus and 3' untranslated region of mouse SphK1 were used as probes for hybridization. The two antisense probes produced the same staining pattern. Sense probes did not show any specific signals.

TUNEL assay. The terminal deoxynucleotidyltransferase-mediated dUTP-biotin nick end labeling (TUNEL) assay was performed with the Tdt-FragEL DNA Fragmentation Detection Kit (Calbiochem) according to the manufacturer's instructions.

Statistics. Data are expressed as means ± standard errors (SE). Results having P values of <0.01, or <0.05 by the paired Student t test, were considered significant.


   RESULTS
Top
 Abstract
 Introduction
 Materials and Methods
 Results
Discussion
 References
 
Targeted disruption of SphK2. We created a null allele of SphK2 by replacing it with a LacZ-Neo cassette (Fig. 1A). By intercrossing heterozygous mutant mice, viable homozygous SphK2 mutant mice were obtained in the expected Mendelian ratio, indicating that this genotype was not associated with embryonic lethality. Correct targeting and deletion in the SphK2 gene were confirmed by Southern blot (Fig. 1B) and PCR (data not shown) analyses of genomic DNA. The absence of SphK2 transcripts from the deleted region in DNA from several tissues of adult homozygous mutant mice was confirmed by RT-PCR (Fig. 1C). Furthermore, no expression of SphK2 protein was detected in lysates of adult tissues derived from SphK2 homozygous mutant mice, as determined by immunoblotting with an SphK2-specific antibody (data not shown). The levels of SphK1 mRNA from several tissues (brain, heart, lung, liver, spleen, kidney, and skeletal muscle) of SphK2 homozygous mutant mice were not significantly different from the levels of that from wild-type mice, as determined by real-time PCR (data not shown). The homozygous SphK2 mutant mice were fertile and had normal longevity: histological analysis of major organs failed to reveal any obvious differences from wild-type mice.

SphK1–/– SphK2–/– mice are not viable. The absence of abnormal gross or histological phenotypes in both SphK1 and SphK2 knockout mice led us to examine the effects of a combined loss of both SphK1 and SphK2. Mice lacking one to four SphK1 and SphK2 alleles were generated by intercrossing SphK1+/– SphK2+/– mice. Offspring lacking one to three SphK alleles in any combination were indistinguishable from the wild type, but no animals lacking all four alleles were born, indicating that the SphK1–/– SphK2–/– genotype was lethal in these embryonic mice. To determine when SphK1–/– SphK2–/– mice die, SphK1+/– SphK2–/– mice were intercrossed and resulting embryos were examined. Between E9.5 and E10.5, SphK1+/+ SphK2–/–, SphK1+/– SphK2–/–, and SphK1–/– SphK2–/– embryos were represented in the expected Mendelian ratio. SphK1–/– SphK2–/– embryos were grossly normal at E9.5; however, by E11.5 and E12.5, all embryos exhibited cranial hemorrhage and none survived beyond E13.5, indicating that expression of either SphK1 or SphK2 is essential for viability. Total SphK activity and S1P levels were measured in homogenates of whole embryos at E11.5. SphK activity and S1P levels were partially reduced in SphK1–/– SphK2+/+ and SphK1+/+ SphK2–/– embryos (Fig. 2A to C). In contrast, there was no detectable phosphorylation of sphingosine in SphK1–/– SphK2–/– embryos, irrespective of whether sphingosine was added in the presence of Triton X-100 (Fig. 2A), which stimulates SphK1 and inhibits SphK2, or as a complex with BSA, a condition in which both SphK1 and SphK2 are normally active (Fig. 2B). Accordingly, S1P levels in SphK1–/– SphK2–/– embryos were not detectable (Fig. 2C). Sphingosine levels in these embryos were not significantly different than levels in wild-type embryos (Fig. 2D), indicating that the lethal defects did not result from an increase in sphingosine. The expression of S1P1, S1P2, and S1P3 mRNAs from SphK1–/– SphK2–/– embryos at E11.5 was not significantly changed from that from control embryos, as determined by real-time PCR (data not shown).


Figure 2
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  		FIG. 2. Measurement of SphK activity and S1P levels in SphK1 SphK2 combined mutants. (A and B) SphK enzymatic activity was determined in wild-type and SphK1–/– SphK2+/+, SphK1+/+ SphK2–/–, and SphK1–/– SphK2–/– mutant embryos at E11.5. The assay was performed in the presence of Triton X-100 (A) or in BSA complexes without Triton X-100 (B). The data represent means ± SEs (n = 3; *, P < 0.01; **, P < 0.05 [paired t test compared with the wild type]). (C) S1P levels in wild-type and SphK1–/– SphK2+/+, SphK1+/+ SphK2–/–, and SphK1–/– SphK2–/– mutant embryos at E11.5. The data represent means ± SEs (n = 3; **, P < 0.05 [paired t test compared with the wild type]) (D) Sphingosine levels in wild-type and SphK1–/– SphK2–/– mutant embryos at E11.5. The data represent means ± SEs (n = 3).

 
Vascular defects. By intercrossing SphK1+/– SphK2–/– mice, SphK1–/– SphK2–/– embryos were obtained in the expected Mendelian frequency, remaining grossly normal at E9.5. At E11.5, cranial hemorrhaging was evident in almost all SphK1–/– SphK2–/– embryos and 17% were not viable (Fig. 3A and B). Severely affected embryos had widespread hemorrhaging in areas other than the brain, such as the spinal cord and mandible (Fig. 3C). Some embryos had developed pericardial hemorrhages (Fig. 3D and H). Histological evaluation at E11.5 revealed that hemorrhaging was principally observed in the cranial mesenchymal region (Fig. 3E and F), sometimes accompanied by intraventricular hemorrhages in the brain (Fig. 3G). By E12.5, most of the SphK1–/– SphK2–/– embryos (70%) had died, apparently because of severe bleeding throughout the body. No embryos survived beyond E13.5.


Figure 3
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  		FIG. 3. Vascular defects in SphK1–/– SphK2–/– mutants. (A to D) Photomicrographs of E11.5 embryos. SphK1–/– SphK2–/– mutant embryos show hemorrhages in the brain (B to D), mandible (B), and spinal cord (C), sometimes along with enlargement of the cardiac profile (D). (E to H) H&E staining of sagittal sections from SphK1–/– SphK2–/– mutant embryos at E11.5. (E and F) Hemorrhage in the cranial mesenchymal region (arrows). (G) Intraventricular hemorrhage (arrow). (H) Pericardial hemorrhage (arrows). FV, fourth ventricle; Ht, heart; LV, lateral ventricle; Mes, mesenchyme; NE, neuroepithelium; TE, telencephalon; RE, rhombencephalon. (I to L) Vascular smooth muscle defects in SphK1–/– SphK2–/– mutants at E11.5. (I and K) H&E staining of sagittal sections of the dorsal aorta. The arrows in panel I and K indicate the wall of the aorta. (J and L) Transverse sections of the dorsal aorta stained with anti-smooth muscle {alpha}-actin (SM{alpha}A). (M to P) Electron microscopic analysis of blood vessels from the capillaries in the cranial mesenchymal region from E11.5 wild-type (M and N) and SphK1–/– SphK2–/– mutant (O and P) embryos. The arrows in panel O indicate broken endothelial cells. BC, blood cell; EC, endothelial cell; EJ, endothelial cell-cell junction; PC, pericyte; Vac, vacuole. Magnifications: M, x1,600; N, x50,000; O and P, x2,000. (Q to T) Whole-mount immunostaining with anti-PECAM-1 antibody of blood vessels in the brains of E10.5 wild-type (Q and R) and SphK1–/– SphK2–/– mutant (S and T) embryos. Note the dilated blood vessels (arrows in panel S) and aberrant network (arrowheads in panel T). Scale bars represent 200 µm (E, F, G, H, I, and K) and 50 µm (J and L).

 
The wall of the dorsal aorta was poorly developed in SphK1–/– SphK2–/– embryos at E11.5, compared to that of wild-type embryos (Fig. 3I and K). This finding led us to examine aortal covering by vascular smooth muscle cells, which is normally complete by E11.5. Visualization of smooth muscle {alpha}-actin revealed that covering of the aorta in SphK1–/– SphK2–/– embryos was patchy and incomplete (Fig. 3L), whereas aortal covering in the wild type was complete (Fig. 3J).

The blood vessel defects in SphK1–/– SphK2–/– embryos were further analyzed by electron microscopy. Endothelial cells were severely defective in all blood vessels in the mesenchymal region of the head (Fig. 3O). Some vessels contained endothelial cells with vacuoles (Fig. 3P). In sharp contrast, endothelial cells in the neuroepithelium were intact in the mutants (data not shown). These findings are compatible with the histological localization of the main focus of bleeding in the mesenchyme. Wild-type endothelial cells were completely intact, having endothelial cell-cell junctions and supportive pericytes (Fig. 3M and N).

To further examine the vascular system in these mutants, whole-mount immunostaining was performed with an antibody directed against platelet endothelial cell adhesion molecule 1 (anti-PECAM-1). In SphK1–/– SphK2–/– embryos at E10.5, remodeling defects of blood vessels in the head were apparent; enlarged, dilated blood vessels (Fig. 3S) had formed, along with an aberrant anastomotic network (Fig. 3T).

Taken together, these results were strongly reminiscent of phenotypes observed in S1P1 receptor-null embryos and in embryos carrying multiple S1P receptor mutations (1, 14, 18), substantiating that the effect of S1P receptors on vascular development is mediated by the S1P ligand.

NTDs. An unexpected finding in SphK1–/– SphK2–/– embryos was exencephaly, a cranial neural tube defect (NTD), at frequencies of 18% at E10.5, 13% at E11.5, and 20% at E12.5 (Fig. 4A to D and data not shown). However, no spina bifida was observed, indicating that the anterior neural tube closure was impaired in these embryos. To further investigate this phenomenon, we examined the expression of SphK1 and SphK2 in embryos at E10.5 by in situ hybridization and X-Gal staining, respectively. SphK1 was expressed in the whole brain, with the highest levels in the telencephalon (Fig. 4E). The expression of SphK2 was relatively ubiquitous, with the strongest signals detected in the limb buds, eyes, and branchial arches, and a weaker, but very apparent, level of expression in the telencephalon and spinal cord (Fig. 4F). These expression patterns overlapped that of the S1P1 receptor, which was most prominent in the telencephalon and heart (18, 22) (Fig. 4G). No staining was detected in control embryos (Fig. 4H and data not shown). These overlapping expression patterns are consistent with the hypothesis that SphK1, SphK2, and the S1P1 receptor are involved in neural development.


Figure 4
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  		FIG. 4. NTDs in SphK1–/– SphK2–/– mutants. (A to D) Exencephaly in SphK1–/– SphK2–/– mutant embryos. (A and B) Wild-type control embryos at E10.5. (C and D) SphK1–/– SphK2–/– mutant embryos at E10.5. (A and C) Lateral view. (B and D) Dorsal view. Ex, exencephaly. (E to H) Expression of SphK1, SphK2, and S1P1 in E10.5 embryos. (E) Whole-mount in situ hybridization for SphK1 in a wild-type embryo. (F, G, and H) Whole-mount X-Gal staining of SphK2–/– and S1P1–/– mutant and wild-type embryos, respectively. The lacZ reporter gene was inserted into the SphK2 and S1P1 loci. TE, telencephalon.

 
The effect of S1P on neural development is antiapoptotic and progrowth. We investigated the mechanism that underlies the NTDs in SphK1–/– SphK2–/– embryos. An imbalance between proliferation and cell survival in the neuroepithelium could potentially cause NTDs, leading to exencephaly (4, 6, 10, 28). S1P has been found to regulate cell growth and survival (8, 24). Therefore, we studied cell survival and growth in the neuroepithelium. Apoptosis was assessed in SphK1–/– SphK2–/– and wild-type embryos at E9.5 and E11.5 by the TUNEL assay. At E9.5, SphK1–/– SphK2–/– embryos showed enhanced apoptosis in the neuroepithelium in the mesencephalon and rhombencephalon, suggesting that this phenomenon may be responsible for the NTDs (Fig. 5A to D). A histological evaluation of the brain revealed a very thin, poorly developed wall of neuroepithelium, along with ventricular dilatation, in SphK1–/– SphK2–/– embryos at E11.5 (Fig. 5E and F). The neuroepithelial layer was irregularly shaped in the whole brain (Fig. 5G and H). Massive cell loss was also found in the neuroepithelial layer (data not shown). These defects were completely penetrative in SphK1–/– SphK2–/– embryos at E11.5, suggesting that the impairment of neural development is a general feature in SphK1–/– SphK2–/– embryos, whether or not exencephaly is present. SphK1–/– SphK2–/– embryos at E11.5 exhibited dramatically increased numbers of apoptotic cells in the neuroepithelium of almost all brain regions, but particularly in the telencephalon, correlating with the dramatic thinning of the neuroepithelial layer (Fig. 5I to K). Cell proliferation was assessed by anti-phospho-histone H3 immunostaining at E11.5. The total number of mitotic cells was significantly decreased in the telencephalon regions of the mutants' brains (Fig. 5L to N), while the number was not significantly changed in the diencephalon and rhombencephalon (Fig. 5N). Together, these results imply that S1P has antiapoptotic and progrowth effects during neural development.


Figure 5
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  		FIG. 5. Increased cell death and decreased cell proliferation in SphK1–/– SphK2–/– mutants. (A and B) H&E staining of transverse sections from wild-type (A) and SphK1–/– SphK2–/– mutant (B) embryos at E9.5. An arrow in panel B indicates an NTD. (C and D) TUNEL assay of wild-type (C) and SphK1–/– SphK2–/– mutant (D) embryos at E9.5. The boxed areas in panels A and B are shown, respectively. NE, neuroepithelium; Mes, mesenchyme. (E to H) H&E staining of sections from wild-type (E and G) and SphK1–/– SphK2–/– mutant (F and H) embryos at E11.5. (E and F) Sagittal sections. (G and H) Transverse sections. DE, diencephalon; FV, fourth ventricle; ME, mesencephalon; RE, rhombencephalon; TE, telencephalon; TV, third ventricle. (I and J) TUNEL assay of wild-type (I) and SphK1–/– SphK2–/– mutant (J) embryos at E11.5. The telencephalon is shown. (K) Percentage of TUNEL-positive cells (n = 5 matched pairs; *, P < 0.01 [paired t test]). (L and M) Immunostaining with anti-phospho-histone H3 of wild-type (L) and SphK1–/– SphK2–/– mutant (M) embryos at E11.5. The telencephalon is shown. (N) Percentage of phospho-histone H3-positive cells (n = 4 matched pairs; *, P < 0.01 [paired t test]). Scale bars represent 500 µm (A, B, E, F, G, and H) and 50 µm (C, D, I, J, L, and M).

 
Requirement of S1P1 receptor for neural development. The expression pattern of the S1P1 receptor implies a role in neural development. Histological analysis of S1P1 receptor-null (S1P1–/–) embryos at E12.5 revealed massive cell loss in the forebrain (Fig. 6A and B). TUNEL analysis showed that apoptotic cells were significantly more numerous in the neuroepithelial layers of the telencephalon and diencephalon regions in S1P1–/– embryos at E12.5 (Fig. 6C to E). A smaller, but significant, increase in cell death was observed in earlier E11.5 S1P1–/– embryos, when bleeding was not evident (data not shown). Cell proliferation was also affected in S1P1–/– embryos at E12.5; mitotic cell numbers were significantly decreased in the telencephalon regions (Fig. 6F to H). These results indicate that the effect of S1P on neural development is likely mediated, at least in part, by signaling from the S1P1 receptor.


Figure 6
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  		FIG. 6. Requirement of S1P1 receptor for neural development. (A and B) H&E staining of transverse sections from wild-type (A) and S1P1–/– mutant (B) embryos at E12.5. (C and D) TUNEL assay of wild-type (C) and S1P1–/– mutant (D) embryos at E12.5. (E) Percentage of TUNEL-positive cells (n = 6 matched pairs; *, P < 0.01; **, P < 0.05 [paired t test]). (F and G) Immunostaining with anti-phospho-histone H3 of wild-type (F) and S1P1–/– mutant (G) embryos at E12.5. (H) Percentage of phospho-histone H3-positive cells (n = 6 matched pairs; *, P < 0.01 [paired t test]). Scale bars represent 200 µm (A, B, C, and D) and 50 µm (F and G).

 

   DISCUSSION
Top
 Abstract
 Introduction
 Materials and Methods
 Results
 Discussion
References
 
We demonstrate that S1P signaling during embryonic development is critical for neurogenesis, in addition to angiogenesis. Simultaneous disruption of the two known sphingosine kinase genes in mice, SphK1 and SphK2, resulted in a deficiency of S1P, which severely disturbed both angiogenesis and neurogenesis, including neural tube closure, followed by embryonic lethality. S1P levels were also partially reduced in SphK1–/– SphK2+/+ and SphK1+/+ SphK2–/– embryos, suggesting that S1P levels are regulated by both SphK1 and SphK2 during development. In contrast, S1P levels in most tissues from SphK1 single-mutant mice were not markedly decreased, although there was a significant reduction (50%) of the S1P level in serum (3). We did not detect a significant reduction of the S1P level in serum from SphK2 single-mutant mice (6 to 8 weeks old).

The vascular defects were expected, since mice with disrupted S1P receptor genes had shown similar defects in vascular development (1, 14, 18). Thus, our findings provide confirmation that the effect of S1P receptors on vascular development is mediated via S1P signaling. In contrast to the vascular defects, neural defects were unexpected and provided an entirely novel insight into the function of S1P signaling during development. About 15 to 20% of SphK-null mice exhibited NTDs, which are prevalent birth defects. More than 80 mutations that cause NTDs in mice have been reported, and alterations in cell survival and cell proliferation are frequently relevant to the NTDs (6). Indeed, our mutant mice showed increased cell death during neural tube closure periods, which may account for the NTDs. It has been reported that fumonisins, toxic and carcinogenic mycotoxins, disrupt sphingolipid metabolism and cause a high incidence of NTDs in mouse embryos in culture (20). It is noteworthy that substantial consumption of fumonisins is correlated with high incidences of NTDs in some regions of the world (20), indicating that disturbance of sphingolipid metabolism may be implicated in the pathogenesis of human NTDs. Thus, our mutant mice might be valuable animal models for common human NTDs.

The SphK-null mice revealed increased cell death and decreased cell proliferation in the neuroepithelial layer, with complete penetrance, even after neural tube closure periods, suggesting that those are general features induced by S1P-deficiency, irrespective of the presence of NTDs. It has been proposed that the effects of S1P on proliferation and suppression of apoptosis are mediated by both intracellular actions and S1P receptors (16, 23, 26, 27). Our results suggest that the effects of S1P on neural development are mediated, at least in part, by the S1P1 receptor. The neural defects, demonstrated by increased cell death and decreased proliferation, in S1P1–/– embryos were milder than those seen in SphK1–/– SphK2–/– embryos. Moreover, in contrast to SphK1–/– SphK2–/– embryos, we did not observe NTDs in S1P1–/– embryos. These results indicate that perhaps other S1P receptors (S1P2 to S1P5) may be important participants in this pathway or that S1P may also act through an intracellular mechanism. Mice carrying multiple S1P receptor mutant alleles, such as S1P1–/– S1P2–/– and S1P1–/– S1P3–/– embryos, die earlier and show more severe vascular defects than do S1P1 single mutants (14). It will be of interest to determine if the S1P receptors have synergistic effects on neurogenesis by analyzing the multiple S1P receptor mutants in more detail.

In summary, these findings demonstrate, for the first time, that S1P plays a critical role in neurogenesis during development through potent effects on neural cell survival and growth. It is noteworthy that S1P, clearly an angiogenic factor, is now implicated in neurogenesis, since it has been recently recognized that the two pathways, angiogenesis and neurogenesis, utilize some of the same molecules for their regulation (30). Furthermore, our findings raise the possibility that manipulation of the S1P/S1P receptor signaling pathway in the nervous system may provide novel therapeutic approaches in neurological disease through enhancement of neuronal survival, increasing proliferation of neural progenitors, or both.


   ACKNOWLEDGMENTS
 
This research was supported by the Intramural Research Program of the NIH, NIDDK, and by NIH grant R 37 GM043880 (to S.S.). K.M. is supported by a JSPS Research Fellowship for Japanese Biomedical and Behavioral Researchers at NIH.

We have no competing financial interests.


   FOOTNOTES
 
* Corresponding author. Mailing address: Genetics of Development and Disease Branch, NIDDK, National Institutes of Health, Bldg. 10, Rm. 9N-314, 10 Center Dr., MSC 1821, Bethesda, MD 20892-1821. Phone: (301) 496-4391. Fax: (301) 496-0839. E-mail: proia{at}nih.gov. Back


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 Abstract
 Introduction
 Materials and Methods
 Results
 Discussion
 References
 
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Molecular and Cellular Biology, December 2005, p. 11113-11121, Vol. 25, No. 24
0270-7306/05/$08.00+0     doi:10.1128/MCB.25.24.11113-11121.2005
Copyright © 2005, American Society for Microbiology. All Rights Reserved.



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