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Open Access Highly Accessed Research article

Glypican-1 controls brain size through regulation of fibroblast growth factor signaling in early neurogenesis

Yi-Huei Linda Jen1, Michele Musacchio2 and Arthur D Lander1*

Author Affiliations

1 Department of Developmental and Cell Biology, Developmental Biology Center and Center for Complex Biological Systems, University of California, Irvine, CA 92697-2300, USA

2 Department of Molecular Biology and Biochemistry, University of California, Irvine, CA 92697-3900, USA

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Neural Development 2009, 4:33  doi:10.1186/1749-8104-4-33


The electronic version of this article is the complete one and can be found online at: http://www.neuraldevelopment.com/content/4/1/33


Received:13 March 2009
Accepted:4 September 2009
Published:4 September 2009

© 2009 Jen et al; licensee BioMed Central Ltd.

This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract

Background

Cell surface heparan sulfate proteoglycans (HSPGs) act as co-receptors for multiple families of growth factors that regulate animal cell proliferation, differentiation and patterning. Elimination of heparan sulfate during brain development is known to produce severe structural abnormalities. Here we investigate the developmental role played by one particular HSPG, glypican-1 (Gpc1), which is especially abundant on neuronal cell membranes, and is the major HSPG of the adult rodent brain.

Results

Mice with a null mutation in Gpc1 were generated and found to be viable and fertile. The major phenotype associated with Gpc1 loss is a highly significant reduction in brain size, with only subtle effects on brain patterning (confined to the anterior cerebellum). The brain size difference emerges very early during neurogenesis (between embryonic days 8.5 and 9.5), and remains roughly constant throughout development and adulthood. By examining markers of different signaling pathways, and the differentiation behaviors of cells in the early embryonic brain, we infer that Gpc1-/- phenotypes most likely result from a transient reduction in fibroblast growth factor (FGF) signaling. Through the analysis of compound mutants, we provide strong evidence that Fgf17 is the FGF family member through which Gpc1 controls brain size.

Conclusion

These data add to a growing literature that implicates the glypican family of HSPGs in organ size control. They also argue that, among heparan sulfate-dependent signaling molecules, FGFs are disproportionately sensitive to loss of HSPGs. Finally, because heterozygous Gpc1 mutant mice were found to have brain sizes half-way between homozygous and wild type, the data imply that endogenous HSPG levels quantitatively control growth factor signaling, a finding that is both novel and relevant to the general question of how the activities of co-receptors are exploited during development.

Background

Cell surface heparan sulfate proteoglycans (HSPGs) have been implicated as key regulators of patterning and growth in animal development [1,2]. Participation in these events is generally thought to reflect their functions as co-receptors for diverse growth factor families, including fibroblast growth factors (FGFs), Wnts, Hedgehogs and bone morphogenetic proteins (BMPs) [3-6]. In both vertebrates and invertebrates, disruption of heparan sulfate biosynthesis leads to severe, pervasive developmental abnormalities. For example, mice completely deficient in heparan sulfate arrest in gastrulation [7].

In contrast, the elimination of the individual core proteins that carry cell surface heparan sulfate generally produces more subtle or tissue-restricted defects, particularly in mammals [8-16]. Most likely this reflects the relatively large number of cell surface HSPGs (six glypicans and four syndecans in mammals), their overlapping patterns of expression, and a likelihood of functional redundancy that is made particularly high by the fact that carbohydrate moieties mediate much of their function. Despite such complexity, the analysis of core protein mutants has provided novel insights into at least some of the developmental and physiological processes in which HSPGs participate.

The glypicans define a structurally conserved family of glycosylphosphatidylinositol-anchored HSPGs that have been extensively studied for their roles in both development and cancer [17-27]. Of the six glypicans in mammals, glypicans 1 and 2 (Gpc1 and Gpc2) were identified early on as major HSPGs of the developing brain [28-31]. Subsequently, Gpc4 and Gpc5 were shown to be regionally expressed in the developing brain as well [32-34]. Biochemical studies suggest that the most abundant glypican in the rodent brain, at least from late gestation onward, is Gpc1 [29,31]. During development, Gpc1 is expressed in both neuroepithelial cells and mature neurons; it is particularly enriched in axons and nerve terminals [35,36]. We reasoned, therefore, that loss of Gpc1 might produce defects in neurogenesis and/or axonal guidance, both of which are driven by growth factors regulated, in many cases, by HSPGs. As described below, the brains of mice rendered null for Gpc1 were morphologically normal, except for subtle mispatterning of the anterior cerebellum, but were abnormally small. Unexpectedly, we found that the reduction in brain size in mutant mice reflects a specific role for Gpc1 at the earliest stages of neurogenesis, before embryonic day (E)9.5.

Results

Generation of glypican-1 null mice

Homologous recombination was used in embryonic stem (ES) cells to flank the first exon of Gpc1 - which includes the translational start site and signal sequence - with loxP sites, and successfully targeted cells were transiently transfected with Cre recombinase to induce excision (Figure 1A). Several independently excised ES clones were injected into C57BL/6 blastocysts to generate chimeric mice, one of which was extensively outcrossed to outbred (CD1; ≥10 generations) and inbred (C57Bl/6; ≥7 generations) mice (Figure 1B). This mutant allele (formally designated Gpc1tm1 Alan) will be referred to here as Gpc1-. A second allele - a gene trap insertion of LacZ into the fourth intron of Gpc1 - will be referred to as Gpc1LacZ.

thumbnailFigure 1. Targeted mutation of the Gpc1 locus creates a null allele. (A) Targeting strategy. A construct was created in which loxP sites flank exon 1 of Gpc1 and FLP recognition target (FRT) sites flank negative (TK) and positive (neo) selection markers. After transfection into embryonic stem (ES) cells, Southern blotting, using a probe located outside the targeted region, permitted verification of targeted integration. Transient tranfection of targeted ES cells with a Cre expression plasmid was then used to remove Gpc1 exon 1 and selection markers, prior to generation of mice. (B) Identification of the Gpc1 wild-type (+) and mutant (-) allele by PCR in mice. (C) Immunoblotting of adult brain membrane fractions with an anti-Gpc1 antibody. The presence of a discrete band found only in samples pretreated with heparitinase (Hase) demonstrates that the immunoreactive molecule is a heparan sulfate proteoglycan (HSPG) core protein. Note the decreased band intensity in heterozygous animals, and complete absence of immunoreactivity in homozygotes. The small apparent difference in mobility and slight tilt of the wild-type band is an artifact of uneven electrophoresis. (D) Immunoblotting of adult brain membrane HSPG core proteins using 3G10 antibody. Notice that the loss of a band at the correct molecular weight for Gpc1 in mutant animals is not accompanied by a substantial, consistent change in the presence of other HSPG cores. Hase, Heparitinase; Case, Condroitinase ABC. (E-G) Whole-mount in situ hybridization for Gpc1 at E8.5. Genotypes are as indicated. Red arrowheads point to areas of high Gpc1 expression in the developing brain and branchial arches. Notice that Gpc1 expression is greatly reduced or absent in homozygous mutants. Levels in heterozygotes are intermediate. (H, I) Whole-mount in situ hybridization for Gpc1 in wild-type (H) and Gpc1-/- (I) embryos at E9.5. Staining has been deliberately overdeveloped to show the absence of signal in the mutant, suggesting that mutant Gpc1 mRNA is unstable. FB, forebrain; HB, hindbrain; MB, midbrain.

Gpc1-/- and Gpc1LacZ/LacZ mice were viable and fertile on outbred and inbred backgrounds, and appeared grossly normal. Biochemical studies revealed a complete absence of Gpc1 core protein from the brains of homozygous Gpc1-/- animals, with intermediate levels in heterozygotes (Figure 1C,D). The expression of other brain heparan sulfate and chondroitin sulfate proteoglycans was not significantly affected (Figure 1D). Immunohistochemistry also demonstrated a loss of Gpc1 staining in both Gpc1-/- and Gpc1LacZ/LacZ mice (not shown). In situ hybridization studies, using both whole embryos and adult brain sections, also revealed a lack of Gpc1 transcripts in Gpc1-/- animals (Figure 1E-I), suggesting that these animals are essentially protein- and message-null.

Loss of glypican-1 leads to reduced brain size and subtle patterning abnormalities of the cerebellum

Gpc1-/- mice were indistinguishable from wild type in gross appearance, size, lifespan, and a variety of simple behaviors (data not shown). Their internal anatomy appeared normal, with the exception of the brain, which was noticeably small (Figure 2A). On the CD1 background, adult Gpc1-/- brains weighed 15.5 ± 1.0% less than wild type, and Gpc1-/+ brains weighed 7.8 ± 1.0% less (Figure 2B). Both results were highly statistically significant, as variation in brain size among individuals within mouse strains is normally very small [37].

thumbnailFigure 2. Adult brain weight from Gpc1 null mutant is significantly reduced. (A) Dorsal views of freshly dissected adult brains. Note the apparent reduction in size of Gpc1-/- brains. (B, C) Wet weights of fresh adult brains. Gpc1 genotypes are as indicated. There is a 15.5% decrease in brain weight in homozygous Gpc1 mutants (P < 0.0001); heterozygotes show an intermediate phenotype (7.8% decrease; * and **P < 0.0001). (B) N = 32 for +/+; 29 for +/-; 36 for -/-. Reduced brain weight is also observed in Gpc1LacZ mutants. (C) N = 9 for +/+; 10 for LacZ/+; 7 for LacZ/LacZ. (D) Body weights of adult Gpc1 mutant and wild-type littermates, grouped by sex. No significant effect of genotype is observed. N = 23 for +/+; 30 for +/-; 37 for -/-. (E) Total DNA content of mutant and wild-type brains was measured as an indication of cell number. The data imply a 20% reduction in Gpc1-/- brains. (*P < 0.001; N = 5 for +/+, and 5 for -/-).

On a C57/Bl6 background, reductions in Gpc1-/- and Gpc1-/+ brain weight were also evident, but less pronounced (11% for Gpc1-/-; data not shown), possibly reflecting the fact that wild-type C57/Bl6 brains are approximately 5% smaller than wild-type CD1 brains to begin with. As shown in Figure 2C, Gpc1LacZ/LacZ mice also displayed reduced brain size (the higher variance of these data likely reflects the mixed CD1/C57 background of these animals). The brain weight reduction did not correlate with sex or body weight in Gpc1- or Gpc1LacZ mutant animals (Figure 2D).

To determine whether changes in brain size were due to the presence of fewer cells or smaller cells, DNA was extracted from whole brains and quantified using Hoechst 33258 fluorescence [38]. As shown in Figure 2E, Gpc1-/- mice had about 20% less DNA per brain than their wild-type littermates. Thus, loss of Gpc1 leads to a 20% decrease in the number of brain cells.

Despite this, the shapes of Gpc1-/- forebrains were morphometrically normal (Additional file 1), and most structures showed no apparent patterning defects. The major exception was found in the gyri of the cerebellar vermis, where the most anterior lobe (lobe I) either did not form or was rudimentary (Figure 3A-F). In addition, the primary fissure was shortened by 12%, with no significant change in the lengths of the other fissures, or in the overall cerebellar perimeter (data not shown). Notably, structures that are disrupted in heparan sulfate-deficient conditional Ext1 mutant mice, such as the interhemispheric commissures and the forebrain septum [39], were present in Gpc1 mutants (Figure 3G-J). In addition, no obvious changes in lamination of the cerebellar or cerebral cortices were observed (Figure 3K-N; and data not shown), and staining for markers of neuronal subpopulations, such as calbindin and parvalbumin, appeared normal (data not shown).

Additional file 1. Morphometric comparison of wild-type and Gpc1-/- forebrains. Freshly dissected adult brains were photographed from the dorsal surface. Tracings of the outline of the forebrain hemispheres were digitized and each curve converted to a series of points, in intervals of 0.03 radians, on a polar plot centered on its centroid. For each genotype, the curves from different brains were overlayed and rotated so that the medial edges of each tracing (which are relatively straight) were optimally aligned. (A) An example from the right hemisphere of nine mutant mice. An average curve was generated by calculating the average distance from the centroid for the family of curves at each angular position. (B) Curves representing one standard deviation above and below the average were similarly produced. (C) A single curve depicting the ratio of the average mutant and wild-type values at each angular position was then generated, and error bars around this curve were calculated from the square root of the sum of the squares of the relative errors (standard deviation/mean) for the two mutant and wild-type average curves; the comparison of nine mutant and four wild-type right hemispheres using this process is shown. The null hypothesis - that mutant and wild-type forebrains are identical in shape - implies that the ratio curve should be a perfect circle (that is, distance to the centroid for mutant and wild-type should differ by the same proportion at every angular position). As shown in (C), a circle (r = 0.937) fit within the error bars at every angular position, implying that mutant forebrains are approximately 6.3% smaller in linear dimension, with no significant difference in forebrain shape. Note that a 6.3% decrease in linear dimension is consistent with an 18% decrease in volume, comparable to the observed 15.5% decrease in total brain weight (Figure 2).

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thumbnailFigure 3. Cerebellar foliation defects in Gpc1 null mice. (A-F) Development of cerebellar foliation. Nissl-stained mid-sagittal sections are shown at postnatal days (P)0, 7 and 27. Lobes I to X are as marked in (H). As early as P7, a loss or severe reduction in folium one (red arrowhead) can be seen in Gpc1-/- mice. (G-J) Forebrain anatomy. Coronal sections at the level of the hippocampus (G, H) and septum (I, J) show that midline commissural tracts appear normal in Gpc1-/- mice. (K-N) Cerebellar lamination. Horizontal sections at P7 (K, L) and P27 (M, N) are shown. The appearance and thickness of the cellular and fiber tract layers are normal in Gpc1-/- mice. CC, corpus callosum; EGL, external granular layer; HC, hipocampal commissure; IGL, internal granular layer; ML, molecular layer; PL, purkinje cell layer; S, septum. Bars in (F, H, J) = 1 mm.

Brain size reduction reflects an early embryonic requirement for Gpc1

Although Gpc1 has been reported to be the major HSPG of the adult brain [35], it is also expressed throughout development of the nervous system, and can be detected in neural tissue as early as head-fold stage (around E7) [35,40]. We therefore measured brain size in Gpc1-/- mice at various developmental stages. At birth, Gpc1-/- brains weighed 15 to 20% less than wild-type brains, that is, they were smaller to about the same degree as seen in adulthood (data not shown). Prior to birth, weights could not be measured accurately given the small size of embryonic brains and the need to dissect under liquid; instead, volumes were estimated from photographic images of fresh embryos (Additional file 2). As shown in Figure 4A-B the estimated volume of Gpc1-/- brains was 22% below that of wild-type littermates as early as E9.5 (Figure 4B). In contrast, brain volumes measured one day earlier (E8.5) exhibited no difference between mutant and wild-type littermate embryos. Apparently, a phenotype of about the same magnitude as seen in adult animals emerges over the course of a single day of development.

Additional file 2. Approaches used for estimation of brain volumes of embryos. Approaches used for estimation of brain volumes of (A) E8.5, (B) E9.5 and (C) E11.5 embryos. Outlines of the primarily neural regions of the head were traced on lateral images of E8.5 to E9.5 embryos, and the enclosed area calculated. At E11.5, separate measurements were made of depth (green line in (C), running from the midbrain-hindbrain boundary (MHB) to the upper nasal-facial junction), height (blue line in (C) connecting the midbrain-forebrain boundary (MFB) to the upper jaw), and width (interocular distance, measured from a frontal view; not shown).

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thumbnailFigure 4. The Gpc1 mutant brain phenotype emerges early in neural development. (A) Lateral images of embryonic day (E)8.5, E9.5 and E11.5 wild-type (+/+) and Gpc1-/- (-/-) embryos. Because the developmental stage of embryos is highly variable at E8.5 to E9.5, not every image is fully representative of the average for that genotype (for quantitative data, see (B, C) below). (B) Gpc1-/- embryos display smaller brains starting at E9.5. Brain size was estimated from photographic images, as described in Additional file 2. Averages of estimated cranial area (at E8.5 and E9.5) and cranial volume (E11.5) were obtained for wild-type and homozygous mutant embryos in multiple litters (N = 23 for +/+ and N = 15 for -/- at E8.5; N = 25 for +/+ and N = 22 for -/- at E9.5; N = 10 for +/+ and N = 18 for -/- at E11.5). Units are pixels2 (× 104) and pixels3 (× 106) for area and volume measurements, respectively. Note the 14.1% decrease in area (* and **P < 0.05) that emerges at E9.5 (consistent with an approximately 20.4% decrease in volume). (C) Comparison of cranial area with somite number in E8.5 and E9.5 wild-type (+/+) and Gpc1-/- (-/-) embryos. Linear regression lines demonstrate that, even when variation in somite number is controlled for, Gpc1-/- brains are of normal size at E8.5, and abnormally small at E9.5. (D-F) Quantification of cell proliferation in the embryonic brain. Sagittal sections of E9.5 embryos were immunostained for phosphohistone H3 (PHH3) (D), counterstained with bizbenzamide (E) and the two images merged (F). Note the concentration of labeled cells along the pial and ventricular margins of the neuroepithelium (outlined). (G, H) Sets of serial sections were stained in this manner from multiple wild-type and Gpc1-/- embryos at E8.5 (N = 5 for both +/+ and -/-), E9.5 (N = 8 for +/+ and N = 7 for -/-), and E11.5 (N = 7 for +/+ and N = 6 for -/-), and numbers of PHH3-labeled cells within the neuroepithelium were counted and normalized to neuroepithelial area for either the entire embryo (G) or the forebrain alone (H). The data show a statistically significant (*P < 0.001) decrease in PHH3-labeling index at E9.5, but no change at E11.5.

To test whether the smaller brain size of E9.5 mutant embryos is a consequence of general developmental delay, we plotted brain size against somite number, a marker of developmental stage (Figure 4C). The data showed a slight trend - which was not statistically significant - toward Gpc1-/- embryos being delayed by about 1 somite (at E8.5, wild type = 11.5 ± 2.8 and mutant = 10.3 ± 3.2; at E9.5, wild type = 22.0 ± 2.4 and mutant = 21.2 ± 2.4). Even taking such a trend into account, regression analysis showed that >70% of the brain size difference at E9.5 is independent of somite number (note the downward shift of the regression line at E9.5). These data suggest that, between E8.5 and E9.5, Gpc1 plays a specific and important role in nervous system growth.

To test whether that role involves regulation of cell proliferation, we used phospho-histone H3 immunohistochemistry to quantify the density of cells in M-phase (Figure 4D-H). If one considers the early central nervous system as a mass of cycling cells undergoing exponential expansion, with a typical cell cycle time of about 8 hours [41,42], then in order to produce a 20% reduction in cell mass over the course of one day of development (and no further decrease thereafter), one would need to lengthen the cell cycle during that day by about 7%. Thus, in Gpc1-/- embryos, we initially expected to see up to an approximately 7% decrease in mitotic labeling index at E8.5, followed by a return to normal on the following day.

Interestingly, we observed a larger and longer-lasting change in labeling index. For example, at E9.5, when we expected proliferation to have returned to wild-type levels, the labeling index in mutant brain neuroepithelium was decreased by 30% (Figure 4G; P < 0.001) The effect was specific to the neuroepithelial cells of these embryos (Additional file 3), and did eventually disappear (by E11.5; Figure 4H). We considered the possibility that the larger-than expected drop in proliferation in Gpc1-/- embryos was being offset by decreased cell death, but this was not supported by direct measurements. TUNEL staining showed that dying cells are not particularly abundant in the wild-type central nervous system at these stages, and if anything, displayed a trend (not statistically significant) toward being more abundant in the mutant, not less. A likely explanation for the delayed and larger-than-expected drop in neural labeling index became apparent later on, after more information about the probable mechanism of GPC1 action was obtained (see below).

Additional file 3. Evaluation of cell proliferation in wild-type (+/+) and Gpc1 mutant (-/-) embryos at E9.5. (A-F) Sagittal sections of E9.5 embryos were immunostained for phosphohistone H3 (PHH3) (A, D), counterstained with bizbenzamide (B, E) and the two images merged (C,F). As quantified in Figure 4G,H, there are fewer PHH3 labeled cells in the Gpc1-/-neuroepithelium than in the wild type. (G) However, as shown here, the PHH3 labeling index specifically in non-neuroepithelial areas of the head is not significantly different between Gpc1-/- and wild-type embryos.

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Redundancy versus compensation within the glypican family

Six structurally similar glypicans are encoded by the mammalian genome. A possible explanation for the relatively mild phenotype in Gpc1-/- mutants would be the participation of other glypicans in the regulation of early embryonic neural proliferation. In fact, Gpc2, Gpc3, Gpc4, Gpc5, and Gpc6 can all be detected in E8.5 and E9.5 embryos, although Gpc3 expression is excluded from most of the nervous system, and Gpc5 is not strongly expressed in brain until later stages (Figure 5A-E) [30,36,40,43]. Interestingly, the expression levels of Glypicans 2 to 6, as judged by whole mount in situ hybridization, were not noticeably altered in Gpc1-/- mutants (Figure 5A-J), suggesting that there is little or no compensatory up-regulation of other glypicans in response to loss of Gpc1. Levels of Gpc4 RNA were also measured by quantitative RT-PCR and were unchanged in Gpc1-/- mice (data not shown).

thumbnailFigure 5. Influences of other glypicans on brain size regulation. (A-J) Whole-mount in situ hybridization for Gpc2, Gpc3, Gpc4, Gpc5 and Gpc6 in E9.5 wild-type (A-E) and Gpc1-/- (F-J) mouse embryos suggests that there is no significant upregulation of other glypicans in response to Gpc1 loss. (K, L) Wet weights of fresh adult brains from allelic combinations of Gpc1- with Gpc2- (K) and Gpc1- with Gpc4lacZ (L). Genotypes are as indicated. The insertion site of the Gpc4LacZ gene-trap allele has not been mapped, precluding development of an allele-specific PCR reaction to distinguish Gpc4LacZ/+ from Gpc4LacZ/LacZ animals. However, since Gpc4 is located on the X chromosome, males with a single LacZ allele are unambiguously hemizygous. Thus, the comparison in (L) is between wild-type (both sexes) and LacZ+ males. Note that Gpc2-/- brains are not significantly different in size from wild type, nor does loss of Gpc2 enhance the phenotype of the Gpc1-/- mouse. In contrast, the Gpc4LacZ mutation significantly enhances the Gpc1-/- phenotype (* and **P < 0.005). N = 7 for Gpc1+/+;Gpc2+/+, N = 5 for Gpc1+/+;Gpc2-/-, N = 3 for Gpc1-/-;Gpc2+/+, N = 3 for Gpc1-/-;Gpc2-/-, N = 2 for Gpc1+/+;Gpc4+/+ and N = 4 for Gpc1+/+;Gpc4+/Y, N = 3 for Gpc1-/-;Gpc4+/+ and N = 8 for Gpc1-/-;Gpc4+/Y, N = 14 for Gpc1+/+;Gpc4Lacz/Y, N = 9 for Gpc1-/-;Gpc4LacZ/Y.

To test for redundancy between Gpc1 and the other glypicans that are expressed in early embryonic brain, we generated double mutants with Gpc2 and Gpc4 (mutants in Gpc6, the third glypican that is strongly expressed in early embryonic brain, have not yet been produced). For Gpc2 we used a targeted allele that, when homozygous, produces phenotypically normal mice with a complete loss of Gpc2 protein (S Saunders and ADL, unpublished data). As shown in Figure 5K, the brains of Gpc2-/- mice are not reduced in size, and the brains of Gpc1-/- ;Gpc2-/- double mutants are no smaller than those of Gpc1-/- mice.

In contrast, when compound mutants were made between Gpc1 and a gene-trap allele of Gpc4 (Gpc4LacZ), brain size appeared synergistically reduced (Figure 5L). This experiment may underestimate the contribution of Gpc4, since the Gpc4LacZ allele is very likely not null (unpublished observations). Thus, within the limits of what can be assessed using existing mutants, Gpc1 appears to act redundantly with at least Gpc4 in controlling brain size.

Evidence for impairment of FGF signaling in the early Gpc1 mutant embryo

Numerous growth factor and morphogen signaling pathways have been implicated in the control of brain growth and development [44-47]. Many of these pathways - including those mediated by Hedgehogs, Wnts, BMPs, and FGFs - are influenced by HSPGs in at least some developmental contexts [1,5,48,49]. To screen for disruption of these pathways in Gpc1-/- mice, we performed in situ hybridization at E8.5 and E9.5 for known downstream markers or reporter genes.

Although we saw no significant differences between wild-type and mutant embryos at these stages in the expression patterns of marker genes for Sonic hedgehog (Shh), BMP and Wnt signaling (Additional file 4), the data suggested that FGF signaling was potentially attenuated. For one marker of FGF signaling - the mitogen-activated protein (MAP) kinase phosphatase Pyst1 (also known as Mkp3 and Dusp6) - we observed no significant change in the Gpc1-/- mouse (Figure 6A-D), but for a second marker - Sprouty 2 (Spry2) - we noticed a consistent, yet transient, reduction in expression. Specifically, Spry2 in situ hybridization was consistently weaker in Gpc1-/- brains at E8.5 to E9.5 (Figure 6E-H), but returned to a near-normal level by E10.25 (Additional file 5). To verify this result, we turned to quantitative RT-PCR. As shown in Figure 6I, there was a 40% reduction in Spry2 mRNA in Gpc1-/- brains at E9.5, with some reduction in Spry1 mRNA (also a FGF target gene) as well. In contrast, and in agreement with the data from in situ hybridization, Pyst1 levels were unchanged.

Additional file 4. Lack of apparent difference in Sonic hedgehog, BMP and Wnt signal intensity in Gpc1-/- during early stages of brain development. (A-J) Whole mount in situ hybridization and reporter gene expression in E8.5 and E9.5 wild type (+/+) and Gpc1-/- (-/-) embryos were used to assess levels and distribution of activity of the Hedgehog, BMP and Wnt signaling pathways, all of which have been reported to be influenced by HSPGs. (A-D) In situ hybridization for Patched1, a marker of Hedgehog signaling. (E-H) In situ hybridization for Msx1, a marker for BMP signaling. Those small differences in staining intensity that are visible in these images (for example, in the anterior hindbrain) were not consistent findings, but reflect a high degree of embryo-to-embryo variability in Msx1 whole mount in situ hybridization. (I-J) β-galactosidase activity in embryos crossed onto a BAT-gal background, in which LacZ expression reports canonical Wnt signaling.

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Additional file 5. Whole mount in situ hybridization for Spry2 at E10.25. When compared with Figure 6E-H, the data suggest that Spry2 expression returns to near-normal in Gpc1-/- embryos by E10.25. These observations are consistent with the view that the disruption of Fgf signaling in Gpc1-/- embryos is transient.

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thumbnailFigure 6. Loss of Gpc1 results in weakened fibroblast growth factor (FGF) signaling and premature neuronal differentiation in brain. (A-D) In situ hybridization for Pyst1. (E-H) In situ hybridization for Sprouty 2 (Spry2). Both are markers of FGF signaling and only for Spry2 was a noticeable change observed between genotypes, with apparent reduced expression in Gpc1-/- embryos at both embryonic day (E)8.5 and E9.5. (I) Real-time quantitative RT-PCR of Pyst1, Spry1 (a third FGF-target gene) and Spry2 from RNA isolated from E9.5 wild-type and Gpc1-/- forebrains. The data imply a significant reduction (32.5%) in Spry2 message levels in the Gpc1 mutant (*P < 0.01), and a possible reduction in Spry1. (J) Erk enzymatic activity was measured by in vitro phosphorylation in E9.5 dorsal forebrain explants from Gpc1+/+ and Gpc1-/- embryos. Such explants display a high level of basal (unstimulated) Erk activity, presumably due to the actions of endogenous growth factors. Erk activity was found to be 41% lower in mutant tissue than in wild type (*P < 0.005; units are cpm × 104). (K, L) Sagittal sections of E9.5 Gpc1+/+ (K) and Gpc1-/- (L) embryos were immunostained with Tuj1 (red), a marker for postmitotic neurons, and counterstained with the nuclear marker bizbenzamide (blue). (K', L') Enlarged images from white boxes in (K) and (L), corresponding to similar locations in the anterior midbrain. Note the greater density of Tuj1-positive cells in the mutant midbrain. White arrowheads in (K, L) point to the ventral forebrain, where virtually no Tuj1-positive cells are found in the wild-type, but several are present in the Gpc1-/- brain. (M, N) Numbers of Tuj1-positive cells within the forebrain (FB) and midbrain (MB) were totaled over serial sections of whole embryos at E8.5 (M) and E9.5 (N). Note the >2-fold increase in Tuj1-positive cells in Gpc1-/- brains at E9.5. In contrast, no significant difference is observed at E8.5. At E9.5, N = 7 for +/+ and N = 4 for -/-; at E8.5, N = 4 for each genotype. *P < 0.005.

To examine FGF signaling more directly, we produced short-term E9.5 dorsal forebrain explant cultures from wild-type and Gpc1-/- embryos, and measured the enzymatic activity of extracellular regulated kinase (ERK) MAP kinase. As shown in Figure 6J, wild-type explants exhibited a high basal level of ERK activity, suggesting a high degree of endogenous growth factor signaling within the explant. In contrast, Gpc1-/- explants exhibited 41% less ERK activity under the same conditions. In response to exogenous FGF2, wild-type explants displayed only a small additional increase in ERK activity, possibly because endogenous signaling was so high. We consistently observed that the exogenous FGF response was even lower in Gpc1-/- explants, but due to the small size of the FGF effect we were unable to establish statistical significance for this conclusion (data not shown). Overall, the data strongly suggest that Gpc1 deficiency diminishes the response of cells of the early nervous system to FGFs.

Loss of glypican-1 results in premature differentiation of postmitotic neurons

It is widely reported that FGFs promote the proliferation of neural progenitor cells [50-59]. In most cases, FGFs appear not to act by affecting cell cycle kinetics, but by increasing the probability that the progeny of dividing cells remain in the cell cycle instead of differentiating (that is, FGFs suppress cell cycle exit). Such a mechanism of FGF action has been established, for example, in the cerebral cortex, the midbrain, the olfactory epithelium and the telencephalic subventricular zone [50,52,53,55,58]. Indeed, even in non-neural tissues such as muscle, preventing cell cycle exit seems to be the central mode of action of FGF [60,61].

If impairment of FGF signaling is the primary mechanism by which Gpc1 deficiency reduces brain size, we reasoned that Gpc1-deficient embryos should exhibit accelerated cell cycle exit and, as a consequence, premature neuronal differentiation. Indeed, this turned out to be the case. As shown in Figure 6K-N, higher than normal numbers of TuJ1+ neurons were detected in the brains of early Gpc1-/- embryos. This effect was especially pronounced at E9.5, when there were over twice as many differentiated neurons in the fore- and midbrains of Gpc1 mutants as in wild-type animals (P < 0.005). To confirm that surplus TuJ1+ neurons were the progeny of cells that had recently undergone cell division, we pulsed embryos at E8.5 with the S-phase label 5-bromo-2'-deoxyuridine (BrdU), and one day later (E9.5) counted the number of TuJ1+/BrdU+ cells in the developing brain. In wild-type embryos we observed an average of 50 ± 3 such cells per mm2, whereas in Gpc1-/- embryos we observed three times as many (150 ± 49; P < 0.05).

Not only do these results support the conclusion that FGF signaling is the main target of Gpc1 in the early central nervous system, they also explain the unexpectedly large, prolonged decreases in mitotic labeling index in Gpc1 mutant embryos (Figure 4G). This is because the labeling index represents the ratio of cells in M phase to total cells. When cells leave the cell cycle, they no longer affect the numerator of this ratio, but still contribute to its denominator, thereby causing an alteration in the labeling index that outlasts, for a period of time, any actual disturbance in the proliferative or differentiative behavior of cells (for a quantitative treatment of this point, see the Supplemental Appendix in Additional file 6). In short, the labeling index data in Figure 4G,H correspond well with the expected consequences of a temporary diminution in activity of a factor, such as FGF, that suppresses the differentiation of neuronal progenitors.

Additional file 6. Supplemental appendix: models for the effect of Gpc1 deficiency on early brain development. Supplemental appendix: models for the effect of Gpc1 deficiency on early brain development

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Glypican-1 acts through Fgf17

Several FGF family members have been implicated in brain development, with the subfamily formed by Fgf8, Fgf17 and Fgf18 having been shown to be especially important at early embryonic stages [44,45,47,62-64]. Fgf8, the most intensively studied of the group, plays critical roles in brain patterning and morphogenesis, and it has been suggested that some of the phenotypes in the Nes-Ext1null brain are the result of impaired Fgf8 function [39]. However, there is substantial overlap in expression of all three of these Fgfs, which also share similar receptor binding properties, and are all thought to control neural proliferation [65-67].

In initial studies of compound mutants involving Gpc1- and Fgf8neo (a hypomorphic allele of Fgf8), we failed to observe significant genetic interaction (that is, a mutant allele of Fgf8 did not further reduce brain weight in a Gpc1 mutant; data not shown). In contrast, we were struck by similarities between the reported defects in anterior cerebellar patterning in Fgf17-/- mice [66] and those reported here for Gpc1 mutants (Figure 3C-F). We therefore generated and analyzed a set of adult Gpc1-;Fgf17- compound mutants (Figure 7).

thumbnailFigure 7. Gpc1 phenotypes require Fgf17. Compound Gpc1/Fgf17 genotypes were produced by interbreeding Gpc1+/-;Fgf17+/- mice. (A-E) Nissl-stained mid-sagittal sections through the cerebella of adult compound mutants. Red arrowheads mark the anterior-most lobe (lobe I), which disappears in both Gpc1-/- and Fgf17-/- animals. Red arrows mark the fusion of lobes III and IV, a phenotype observed in Fgf17-/- mice. Note that the Gpc1-/-;Fgf17-/- phenotype is no more severe than the single Fgf17-/- phenotype. (F) Fresh brain weights of adult compound mutants. Genotypes for each category are as indicated; 'N' refers to the number of animals obtained of each genotype. The data show that, on their own, the presence of either one or two copies of mutant alleles for either Gpc1 or Fgf17 progressively reduces brain size. When animals are null for Fgf17, the presence of mutant Gpc1 alleles has no significant effect (*P < 0.005; **P < 0.001; by Student's t-test).

Representative midline cerebellar morphologies of animals of various compound genotypes are shown in Figure 7A-E. Figure 7F summarizes the distributions of brain weights among the entire collection, by genotype. The data clearly show that, as with Gpc1, loss of wild-type Fgf17 alleles leads to a progressive reduction in brain size and anterior cerebellar defects. Moreover, in animals that possessed either one or two functional Fgf17 alleles, the additional loss of one or two Gpc1 alleles led to a further reduction in brain size. However, in animals null for Fgf17, loss of Gpc1 had no significant phenotypic effect, either on brain size or cerebellar morphology. Complete dependence of the Gpc1 phenotype on the presence of a functional Fgf17 gene provides strong evidence that Fgf17 is, if not the only FGF through which Gpc1 acts, certainly among the most important, at least with respect to the control of brain size and cerebellar patterning.

Discussion

The data presented here establish that Gpc1 plays a role in controlling brain size by regulating the behavior of progenitor cells during early brain development. Although the quantitative effect of Gpc1 loss is modest - a 20% decrease in cell number - it is highly significant when compared to normal variation in brain size within genetically homogeneous mice (Figure 2). The effect appears to be due to a shift in the balance of progenitor cell proliferation versus differentiation over the course of approximately one day of development - from E8.5 to E9.5 (Figures 4 and 6). Diminished signaling by FGFs, but not other growth factors, could be demonstrated at around this time period in Gpc1-/- mice (Figure 6). Genetic epistasis experiments strongly suggested that reduced Fgf17 signaling accounts for most or all of the Gpc1 mutant phenotypes observed here.

The transient and modest effects of Gpc1 loss raised the possibility of either compensation by, or redundancy with, other HSPGs, and although no evidence for compensatory up-regulation of other core proteins was obtained, studies with Gpc1-;Gpc4LacZ double mutants suggested that Gpc1 and Gpc4 may have at least partially overlapping functions in controlling brain size (Figure 5). This idea is lent further support by recent studies in Xenopus, in which morpholino-mediated knockdown of Gpc4 led to a reduction in size of dorsal forebrain structures [68].

It is noteworthy that Gpc1-/- mice failed to display any of the severe developmental phenotypes reported for the Nestin1-Cre mediated conditional inactivation of Ext1, which produces a mouse in which all heparan sulfate is eliminated from the brain from about E10 onward. The phenotypes of the Nes1-Ext1null mouse include specific hypoplasia of the cerebral hemispheres, absence of the cerebellum and olfactory bulbs, and loss of certain midline commissural tracts. It is possible that the mild deficits in the anterior cerebellum that we observed in the Gpc1-/- mouse are related to the cerebellar agenesis seen in the Nes1-Ext1null mouse. Interestingly, even when double mutant mice were made between Gpc1- and Gpc4LacZ (Figure 5), Gpc2- (Figure 5) or Gpc5- (YHJ, ADL and S Saunders, unpublished observations), Nes1-Ext1null phenotypes were not observed. It may be that the combined loss of function of multiple glypicans, and/or glypicans as well as syndecans (the other major family of HSPGs), is required to substantially eliminate heparan sulfate function in brain development.

The growth factor families that have been shown to utilize HSPGs as co-receptors include FGFs, BMPs, Hedgehogs and Wnts [1,3,5,44,69-73] - all of which play important roles during early brain development [74-79]. It was surprising, therefore, that evidence only for reduced FGF signaling was obtained in the Gpc1-/- mouse. Such evidence included reduced expression of FGF target genes, decreased basal Erk activation, and premature neuronal differentiation (Figure 6), as well as genetic epistasis between Gpc1 and Fgf17 (Figure 7). Several of the phenotypes in the Nes1-Ext1null mouse are also consistent with reduced FGF signaling, including cerebellar and olfactory bulb agenesis and cerebral cortical hypoplasia [64,66,80,81]. Diminished FGF signaling has also been implicated in the lens phenotypes in Ndst1 mutant mice (which produce aberrantly sulfated heparan sulfate [82,83]). These observations suggest that, in vivo, FGF signaling may be an especially sensitive indicator of deficits in HSPG function.

A fascinating aspect of the Gpc1 mutant phenotype is that the brain weight of heterozygous animals falls halfway between that of wild type and homozygous mutants (Figure 2). This implies that the amount of Gpc1 expressed by cells influences, in a continuous fashion, the level of growth factor signaling that cells perceive. In other words, Gpc1 may not merely be necessary for growth factor signaling, but a quantitative regulator of the 'gain' of signaling. Accordingly, regulation of Gpc1 expression may be an important part of the control circuitry that keeps brain size so tightly regulated in mammals [37,84].

Recent work suggests a similar quantitative role - albeit in the opposite direction - for Gpc3 [85]. Mouse Gpc3 mutants are known to display marked pre- and postnatal overgrowth of many organs, phenocopying Simpson Golabi Behmel syndrome (a syndrome caused by mutations in human GPC3 [8,9,86]). Because Gpc3 is on the X chromosome, gene dosage effects are not observable with null alleles, but studies of naturally occurring polymorphisms in the Gpc3 regulatory region have recently implied that quantitative variation in the level of Gpc3 expression directly (negatively) controls body size [85]. Even though the molecular mechanism of somatic growth inhibition by Gpc3 is likely to differ from the mechanism of brain growth promotion by Gpc1, the implication of both glypicans in quantitative regulation of size is striking. Intriguingly, a variety of studies in Drosophila also link invertebrate glypicans to organ size control [87-89].

The present study leaves unresolved the role that glypicans play in axons and nerve terminals, where Gpc1 and Gpc2 are especially abundant [36]. The absence of obvious defects in axonal pathways in the Gpc1-/- mouse suggests that these molecules may play more of a role in synaptic physiology than in axonal growth or guidance. Certainly, evidence for the participation of syndecan-2 and syndecan-3 in synapse formation [14,90-92], as well as recent work on the Drosophila nervous system [89,93-95], suggests that HSPGs may play a variety of as yet unappreciated roles in basic neurophysiology. To this end, it is intriguing that recent genome-wide association studies in man have identified both GPC1 and FGFR2 (which encodes a major FGF receptor of the brain) as members of a small handful of genetic loci that correlate with risk of schizophrenia [96,97], a psychiatric disorder also associated with a small, but significant, reduction in brain volume [98,99]. Clearly, a detailed behavioral and neurophysiological examination of the Gpc1 mutant mouse seems warranted in the future.

Conclusion

Cell-surface HSPGs are critical for growth and patterning in numerous tissues and organ systems, presumably as a consequence of their actions as growth factor co-receptors. Here we show that Gpc1 controls the size of the mammalian brain through an unexpectedly specific mechanism: regulation of the proliferation/differentiation behavior of progenitor cells during a very early stage of neurogenesis. We provide evidence that this action is mediated through regulation of Fgf17 signaling, and further show that Gpc1's effects are gene-dosage dependent. The data support the view that glypicans, and possibly HSPGs in general, serve as quantitative regulators of the gain of growth factor signaling during neural development.

Materials and methods

Mice

Gpc1- heterozygous mutants were bred extensively onto CD1 and C57BL/6 backgrounds prior to breeding inter se to produce homozygous mutant animals. PCR primers specific for the Gpc1- allele were 5'-AGCCGGCTTTTGTTGTCTC-3' and 5'-CACGAGTGTGCTAGGATAGGG-3'. Primers specific for the Gpc1 wild-type allele were 5'-CAGCGAAGTCCGCCAGAT-3' and 5'-CAGACCTCCCGAGTGCTAGG-3'.

The following additional mutant alleles were used in this study: gene-trap alleles of Gpc1 (GPC1lacZ; Baygenomics ID GST062 San Francisco, CA, USA) and Gpc4 (GPC4lacZ; Baygenomics ID Ex194) [100,101]; a targeted null mutation in Gpc2 (S Saunders and ADL, unpublished); Fgf2 (Jackson Laboratory, Bar Harbor, Maine, USA), a hypomorphic allele of Fgf8 (Fgf8neo [102]), Fgf17 ([74]) and a LacZ-reporter of canonical Wnt signaling (Bat-gal [103]). Wild type CD1 and C57BL/6 mice were from Charles River (San Diego, CA, USA) Genotypes were determined by PCR of tail DNA.

For production of staged embryos, timed matings were used and noon of the day of vaginal plug was considered as E0.5. At early embryonic stages, more precise staging was obtained from somite number. To obtain BrdU-labeled embryos, pregnant mice were injected intraperitoneally with 50 μg of BrdU (B5002; Sigma-Aldrich St. Louis, MO, USA)per gram body weight and embryos were collected 24 hours later.

Mouse colonies were maintained, and all animal experimentation conducted, in accordance with the policies and guidelines of the Institutional Animal Care and Use Committee (IACUC) of the University of California, Irvine. (IACUC protocol number 1998-1656).

Histology and histochemistry

Adult brains were fast-frozen in 2-methyl-butane prior to cryomicrotome sectioning at 20 μm. Embryos were dissected in cold phosphate-buffered saline (PBS), fixed in 4% paraformaldehyde in PBS at 4°C overnight, cryoprotected in 30% sucrose in PBS at 4°C, and cryomicrotome sectioned at 10 to 20 μm. Sections were stored at -20°C prior to immunohistochemistry or Cresyl-Violet staining. For BrdU staining, cryosections were treated with 2 M HCl for 1 hour at 37°C. Sections were then blocked with 5% goat serum +10% bovine serum albumin/PBS +0.2% Tween20 and incubated with primary antibody diluted in blocking solution at 4°C overnight (anti-Gpc1 [27], 1:500; rabbit anti-phosphohistone H3 (anti-PHH3; Millipore, Billerica, MA, USA, 5 μg/ml, 1:500; Tuj1 (R&D systems, 1:1,000, Minneapolis, MN, USA); anti-BrdU (Abcam, 1:100, Cambridge, MA, USA). Secondary antibodies (alexaFluor goat anti-rabbit IgG, 2 μg/ml alexaFluor goat anti-mouse IgG, 10 μg/ml; Cy3-goat anti mouse, 7 μg/ml (Jackson Immunoresearch, West Grove, PA, USA); or Cy2-goat anti rat, 14 μg/ml (Jackson Immunoresearch)) were applied for 1 hour at room temperature. For quantification of apoptosis, fluorescent TUNEL (terminal deoxynucleotidyl transferase dUTP nick end labeling) assays (Apotag Kit, Serologicals, Norcross, GA, USA) were performed on cyrosections. Hoechst33258 was used at 2 μg/ml for nuclear counterstaining. Fluorescence images were analyzed with a Ziss Axiovert S100 microscope and Hamamatsu C4742-95 digital camera. Wholemount staining for beta-galactosidase activity was performed as described in [104].

In situ hybridization

E8.5-E9.5 embryos, fixed by immersion in 4% paraformaldehyde, were gradually dehydrated in methanol and stored in 100% methanol at -20°C. Wholemount RNA in situ hybridization was performed as described [105] with probes synthesized using digoxigenin-labeled NTP mix (Roche, Indianapolis, IN, USA). Probes for glypicans (Glypicans 1 to 6) were obtained by RT-PCR from E13.5 brain total RNA, using the following primer pairs, and subcloned into the PCRII-TOPO vector (Invitrogen, Carlsbad, CA, USA): Gpc1, 5'-GCTACATCTCCATCTTCCTTGAC-3' and 5'-AACACACATTATCCACTGACACC-3'; Gpc2, 5'-AGTCTGGCGAGGGGTTAGAT-3' and 5'-GGCTACATTGAGGCAGAAGC-3'; Gpc3, 5'-GGATGGTGAAAGTGAAGAATCAAC-3' and 5'-GAGAGAAAGAGAAAAGAGGGAAAC-3'; Gpc4, 5'-CATGGCACGCTTAGGCTTGCTCGC-3' and 5'-TGGTTGCACTGTTCGCTGACCACG-3'; Gpc5, 5'-CGCCAGGATGTTAGTCCATT-3' and 5'-AATTTCTGCCCATTGAGGTG-3'; Gpc6, 5'-GCTGTGTATTCTTGCTCTCTCCGGG-3' and 5'-GTACAGCATCCCGTAGGTCCGGAC-3'.

The following additional RNA probes were used: Pax6 (335 to 595 bp MN_013627), Spry2 (probe used in [106]), Pyst1 (probe used in [107]), Ptc1 (probe used in [108]), Msx1 (EcoRI fragment from IMAGE clone 903377). Controls for in situ hybridization consisted of sense probes derived from the same DNA fragments.

Measurement of brain size and DNA content

Postnatal and adult brains were freshly dissected. After removal of olfactory bulbs and remaining spinal cord (at the level of the posterior margin of the cerebellum), brains were immediately weighed on a laboratory scale.

Images of fresh embryos were collected using a Leica MZFLIII stereomicroscope and a SPOT camera (Diagnostic Instruments, Inc. Sterling Heights, MI, USA). For embryos at E11.5 or older, brain height, depth and width were separately measured from lateral and frontal images (Additional file 2), and multiplied to produce a volume estimate. For E8.5 and E9.5 embryos, measurements of area were obtained from perimeter tracings of lateral views using Image J analysis software [109]. At these stages the central nervous system comprises the majority of head tissue, so such tracings included the entire head, stopping ventrally at the rostral border of the first branchial arch, and dorsally at the top of mesencephalon. Volume was then estimated as area3/2. In some cases, volume was also estimated by the procedures outlined above for older embryos, and qualitatively similar results were obtained.

DNA content in brain homogenates was measured by enhancement of bisbenzimid fluorescence at 458 nm, as described by Labarca and Paigen [38]. A linear standard curve (1 to 10 μg/ml) was obtained using salmon sperm DNA (Invitrogen).

Quantitative RT-PCR

Forebrain vesicles of E9.5 and E8.5 wild-type and mutant mice were dissected in ice-cold PBS, and RNA was isolated and column purified (Aurum Total RNA Mini Kit, Bio-Rad, Herculeus, CA, USA) according to the manufacturer's instructions. cDNA was generated by reverse transcription with a mixture of oligo dT and random hexamers (Superscript First-Strand Synthesis kit, Invitrogen). PCR quality controls, experimental runs and statistical methods were performed as described [110,111]. Quantification of total mRNA expression was performed with an Opticon System (MJ Systems CFD-3200, Calgary, Denver, USA) and SYBR-Green (Bio-Rad).

All measurements were normalized to values for 18S RNA in the same samples. All cDNA samples were validated for reverse transcription reaction efficiency and minimal genomic DNA contamination (cDNA/genomic target ratio >105) for 40 cycles in duplicates. Average of duplicated cycle threshold (Ct) values were normalized as ΔCt (Ctgene of interest - Ctreference(18S)). Relative levels were converted using the 2-ΔΔCt method: ΔΔCt = ΔCtmutant - ΔCtwild-type [112] Averages of duplicate Ct, normalized ΔCt, ΔΔCt and relative level 2-ΔΔCt and standard errors were calculated using Microsoft Excel.

Measurement of Erk activity in embryonic explant cultures

E9.5 dorsal telencephalon explants were isolated and cultured as previously described [110]. After 1 hour of incubation at 37°C, FGF2 (R&D Systems) was added at the concentrations indicated for 15 minutes. Explants were briefly washed with 1× PBS and individually homogenized in lysis buffer (1 mM EGTA, 1% Triton X-100, 150 mM NaCl, 50 mM Tris-Cl pH7.4, 1% NP40, 1 μg/ml phenylmethylsulphonyl fluoride (PMSF), 1 μg/ml leupeptin, 1 μg/ml pepstatin, 1 μg/ml aprotinin, 25 μg/ml N-ethylmaleimide (NEM), and phosphatase inhibitors (1 mM NaF, 1 mM Na3VO4)) with a disposable pestle (Knotes Scientific, Vineland, NJ, USA) Lysed samples were stored at -80°C until use. Erk activity was quantified using an in vitro phosphorylation assay (MAP Kinase/Erk Assay kit; Upstate Biotechnology) following the manufacturer's instructions, with or without the 20 μM Erk inhibitor FR180204 (Calbiochem, Gibbstownm, NJ, USA) treatment for 10 minutes prior to the assay. Values in the presence of FR180204 were taken to represent non-ERK phosphorylation activity, and subtracted from each data point. Data were normalized to protein concentration determined by a bicinchoninic acid (BCA) assay [113].

Subcellular fractionation and analysis of proteoglycan content

Adult brains were dissected in ice-cold PBS and immediately homogenized. to obtain membrane and soluble fractions as described [114]. For SDS-PAGE analysis, samples prepared in this way were digested for 30 minutes at 37°C with Heparinase III or with Heparinase III plus Chondroitinase ABC (all used at 1.5 U/mg of protein; both enzymes were purchased from Seikagaku Corp., Tokyo, Japan) along with a proteinase inhibitor mixture (10 μg/ml pepstatin A, 20 μg/ml leupeptin, 2.5 mg/ml NEM, and PMSF in 50 mM Tris-hydroxyaminomethane, 15 mM phosphoric acid, pH7.3). Digested samples were boiled for 10 minutes in SDS-PAGE sample buffer and loaded at 50 μg protein per lane onto 7.5% SDS-polyacrylamide gels, and subjected to electrophoresis. Gels were transferred to PVDF membrane (Millipore, Billerica, MA, USA) and probed with rabbit anti-glypican-1 (1:3,000) antibody or mouse 3G10 monoclonal antibody (1:2,000; USBiological, Swampscott, MA, USA). Samples without enzyme treatment, or subjected to single enzyme treatment, were used where indicated. Blots were incubated with horseradish peroxidase-conjugated goat anti-rabbit or donkey anti-mouse antibody, as appropriate, and visualized using enhanced chemiluminescence.

Abbreviations

BMP: bone morphogenetic protein; BrdU: 5-bromo-2'-deoxyuridine; E: embryonic day; ERK: extracellular regulated kinase; ES: embryonic stem; FGF: fibroblast growth factor; Gpc: glypican; HSPG: heparan sulfate proteoglycan; MAP: mitogen-activated protein; NEM: N-ethylmaleimide; Spry: Sprouty; PBS: phosphate-buffered saline; PHH3: phosphohistone H3; PMSF: phenylmethylsulphonyl fluoride.

Competing interests

The authors declare that they have no competing interests.

Authors' contributions

YHJ and ADL conceived of the studies, designed the experiments, interpreted the data and wrote the manuscript. YHJ carried out the experiments, except for the generation of Gpc1 knockout mice, which was carried out by MM.

Acknowledgements

We thank Felix Truong, Betty Yeh, and Karishima Datye for their excellent technical assistance and Edwin Monuki and Spencer Currle for their assistance in setting up forebrain explant and quantitative PCR assays. We thank David Ornitz for providing Fgf17 mice, Anne Calof for providing Fgf8neo mice, Maike Sander for BAT-gal mice, and William Skarnes for Gpc1LacZ and Gpc4LacZ mice. This work was supported by NIH grants R01-NS26862 and P50-GM076516.

References

  1. Lin X: Functions of heparan sulfate proteoglycans in cell signaling during development.

    Development 2004, 131:6009-6021. PubMed Abstract | Publisher Full Text OpenURL

  2. Perrimon N, Bernfield M: Specificities of heparan sulphate proteoglycans in developmental processes.

    Nature 2000, 404:725-728. PubMed Abstract | Publisher Full Text OpenURL

  3. Gallagher J: Messages in the matrix: proteoglycans go the distance.

    Dev Cell 2007, 13:166-167. PubMed Abstract | Publisher Full Text OpenURL

  4. Baeg GH, Lin X, Khare N, Baumgartner S, Perrimon N: Heparan sulfate proteoglycans are critical for the organization of the extracellular distribution of Wingless.

    Development 2001, 128:87-94. PubMed Abstract | Publisher Full Text OpenURL

  5. Carrasco H, Olivares GH, Faunes F, Oliva C, Larrain J: Heparan sulfate proteoglycans exert positive and negative effects in Shh activity.

    J Cell Biochem 2005, 96:831-838. PubMed Abstract | Publisher Full Text OpenURL

  6. Paine-Saunders S, Viviano BL, Economides AN, Saunders S: Heparan sulfate proteoglycans retain Noggin at the cell surface: a potential mechanism for shaping bone morphogenetic protein gradients.

    J Biol Chem 2002, 277:2089-2096. PubMed Abstract | Publisher Full Text OpenURL

  7. Stickens D, Zak BM, Rougier N, Esko JD, Werb Z: Mice deficient in Ext2 lack heparan sulfate and develop exostoses.

    Development 2005, 132:5055-5068. PubMed Abstract | Publisher Full Text OpenURL

  8. Paine-Saunders S, Viviano BL, Zupicich J, Skarnes WC, Saunders S: glypican-3 controls cellular responses to Bmp4 in limb patterning and skeletal development.

    Dev Biol 2000, 225:179-187. PubMed Abstract | Publisher Full Text OpenURL

  9. Cano-Gauci DF, Song HH, Yang H, McKerlie C, Choo B, Shi W, Pullano R, Piscione TD, Grisaru S, Soon S, Sedlackova L, Tanswell AK, Mak TW, Yeger H, Lockwood GA, Rosenblum ND, Filmus J: Glypican-3-deficient mice exhibit developmental overgrowth and some of the abnormalities typical of Simpson-Golabi-Behmel syndrome.

    J Cell Biol 1999, 146:255-264. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  10. Stepp MA, Gibson HE, Gala PH, Iglesia DD, Pajoohesh-Ganji A, Pal-Ghosh S, Brown M, Aquino C, Schwartz AM, Goldberger O, Hinkes MT, Bernfield M: Defects in keratinocyte activation during wound healing in the syndecan-1-deficient mouse.

    J Cell Sci 2002, 115:4517-4531. PubMed Abstract | Publisher Full Text OpenURL

  11. Gotte M, Bernfield M, Joussen AM: Increased leukocyte-endothelial interactions in syndecan-1-deficient mice involve heparan sulfate-dependent and -independent steps.

    Curr Eye Res 2005, 30:417-422. PubMed Abstract | Publisher Full Text OpenURL

  12. Gotte M, Joussen AM, Klein C, Andre P, Wagner DD, Hinkes MT, Kirchhof B, Adamis AP, Bernfield M: Role of syndecan-1 in leukocyte-endothelial interactions in the ocular vasculature.

    Invest Ophthalmol Vis Sci 2002, 43:1135-1141. PubMed Abstract | Publisher Full Text OpenURL

  13. Reizes O, Lincecum J, Wang Z, Goldberger O, Huang L, Kaksonen M, Ahima R, Hinkes MT, Barsh GS, Rauvala H, Bernfield M: Transgenic expression of syndecan-1 uncovers a physiological control of feeding behavior by syndecan-3.

    Cell 2001, 106:105-116. PubMed Abstract | Publisher Full Text OpenURL

  14. Kaksonen M, Pavlov I, Voikar V, Lauri SE, Hienola A, Riekki R, Lakso M, Taira T, Rauvala H: Syndecan-3-deficient mice exhibit enhanced LTP and impaired hippocampus-dependent memory.

    Mol Cell Neurosci 2002, 21:158-172. PubMed Abstract | Publisher Full Text OpenURL

  15. Echtermeyer F, Streit M, Wilcox-Adelman S, Saoncella S, Denhez F, Detmar M, Goetinck P: Delayed wound repair and impaired angiogenesis in mice lacking syndecan-4.

    J Clin Invest 2001, 107:R9-R14. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  16. Wilcox-Adelman SA, Denhez F, Goetinck PF: Syndecan-4 modulates focal adhesion kinase phosphorylation.

    J Biol Chem 2002, 277:32970-32977. PubMed Abstract | Publisher Full Text OpenURL

  17. Stringer SE, Gallagher JT: Heparan sulphate.

    Int J Biochem Cell Biol 1997, 29:709-714. PubMed Abstract | Publisher Full Text OpenURL

  18. David G, Bernfield M: The emerging roles of cell surface heparan sulfate proteoglycans.

    Matrix Biol 1998, 17:461-463. PubMed Abstract | Publisher Full Text OpenURL

  19. Alexander CM, Reichsman F, Hinkes MT, Lincecum J, Becker KA, Cumberledge S, Bernfield M: Syndecan-1 is required for Wnt-1-induced mammary tumorigenesis in mice.

    Nat Genet 2000, 25:329-332. PubMed Abstract | Publisher Full Text OpenURL

  20. Blackhall FH, Merry CL, Davies EJ, Jayson GC: Heparan sulfate proteoglycans and cancer.

    Br J Cancer 2001, 85:1094-1098. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  21. De Cat B, David G: Developmental roles of the glypicans.

    Semin Cell Dev Biol 2001, 12:117-125. PubMed Abstract | Publisher Full Text OpenURL

  22. Filmus J, Selleck SB: Glypicans: proteoglycans with a surprise.

    J Clin Invest 2001, 108:497-501. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  23. Song HH, Filmus J: The role of glypicans in mammalian development.

    Biochim Biophys Acta 2002, 1573:241-246. PubMed Abstract | Publisher Full Text OpenURL

  24. Kramer KL, Yost HJ: Heparan sulfate core proteins in cell-cell signaling.

    Annu Rev Genet 2003, 37:461-484. PubMed Abstract | Publisher Full Text OpenURL

  25. Hacker U, Nybakken K, Perrimon N: Heparan sulphate proteoglycans: the sweet side of development.

    Nat Rev Mol Cell Biol 2005, 6:530-541. PubMed Abstract | Publisher Full Text OpenURL

  26. Ding K, Lopez-Burks M, Sanchez-Duran JA, Korc M, Lander AD: Growth factor-induced shedding of syndecan-1 confers glypican-1 dependence on mitogenic responses of cancer cells.

    J Cell Biol 2005, 171:729-738. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  27. Aikawa T, Whipple CA, Lopez ME, Gunn J, Young A, Lander AD, Korc M: Glypican-1 modulates the angiogenic and metastatic potential of human and mouse cancer cells.

    J Clin Invest 2008, 118:89-99. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  28. Karthikeyan L, Maurel P, Rauch U, Margolis RK, Margolis RU: Cloning of a major heparan sulfate proteoglycan from brain and identification as the rat form of glypican.

    Biochem Biophys Res Commun 1992, 188:395-401. PubMed Abstract | Publisher Full Text OpenURL

  29. Karthikeyan L, Flad M, Engel M, Meyer-Puttlitz B, Margolis RU, Margolis RK: Immunocytochemical and in situ hybridization studies of the heparan sulfate proteoglycan, glypican, in nervous tissue.

    J Cell Sci 1994, 107:3213-3222. PubMed Abstract | Publisher Full Text OpenURL

  30. Stipp CS, Litwack ED, Lander AD: Cerebroglycan: an integral membrane heparan sulfate proteoglycan that is unique to the developing nervous system and expressed specifically during neuronal differentiation.

    J Cell Biol 1994, 124:149-160. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  31. Litwack ED, Stipp CS, Kumbasar A, Lander AD: Neuronal expression of glypican, a cell-surface glycosylphosphatidylinositol-anchored heparan sulfate proteoglycan, in the adult rat nervous system.

    J Neurosci 1994, 14:3713-3724. PubMed Abstract | Publisher Full Text OpenURL

  32. Saunders S, Paine-Saunders S, Lander AD: Expression of the cell surface proteoglycan glypican-5 is developmentally regulated in kidney, limb, and brain.

    Dev Biol 1997, 190:78-93. PubMed Abstract | Publisher Full Text OpenURL

  33. Hagihara K, Watanabe K, Chun J, Yamaguchi Y: Glypican-4 is an FGF2-binding heparan sulfate proteoglycan expressed in neural precursor cells.

    Dev Dyn 2000, 219:353-367. PubMed Abstract | Publisher Full Text OpenURL

  34. Watanabe K, Yamada H, Yamaguchi Y: K-glypican: a novel GPI-anchored heparan sulfate proteoglycan that is highly expressed in developing brain and kidney.

    J Cell Biol 1995, 130:1207-1218. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  35. Litwack ED, Ivins JK, Kumbasar A, Paine-Saunders S, Stipp CS, Lander AD: Expression of the heparan sulfate proteoglycan glypican-1 in the developing rodent.

    Dev Dyn 1998, 211:72-87. PubMed Abstract | Publisher Full Text OpenURL

  36. Ivins JK, Litwack ED, Kumbasar A, Stipp CS, Lander AD: Cerebroglycan, a developmentally regulated cell-surface heparan sulfate proteoglycan, is expressed on developing axons and growth cones.

    Dev Biol 1997, 184:320-332. PubMed Abstract | Publisher Full Text OpenURL

  37. Williams RW: Mapping genes that modulate mouse brain development: a quantitative genetic approach.

    Results Probl Cell Differ 2000, 30:21-49. PubMed Abstract OpenURL

  38. Labarca C, Paigen K: A simple, rapid, and sensitive DNA assay procedure.

    Anal Biochem 1980, 102:344-352. PubMed Abstract | Publisher Full Text OpenURL

  39. Inatani M, Irie F, Plump AS, Tessier-Lavigne M, Yamaguchi Y: Mammalian brain morphogenesis and midline axon guidance require heparan sulfate.

    Science 2003, 302:1044-1046. PubMed Abstract | Publisher Full Text OpenURL

  40. Luxardi G, Galli A, Forlani S, Lawson K, Maina F, Dono R: Glypicans are differentially expressed during patterning and neurogenesis of early mouse brain.

    Biochem Biophys Res Commun 2007, 352:55-60. PubMed Abstract | Publisher Full Text OpenURL

  41. Kauffman SL: An autoradiographic study of the generation cycle in the ten-day mouse embryo neural tube.

    Exp Cell Res 1966, 42:67-73. PubMed Abstract | Publisher Full Text OpenURL

  42. Gressens P, Paindaveine B, Hill JM, Evrard P, Brenneman DE: Vasoactive intestinal peptide shortens both G1 and S phases of neural cell cycle in whole postimplantation cultured mouse embryos.

    Eur J Neurosci 1998, 10:1734-1742. PubMed Abstract | Publisher Full Text OpenURL

  43. Ybot-Gonzalez P, Copp AJ, Greene ND: Expression pattern of glypican-4 suggests multiple roles during mouse development.

    Dev Dyn 2005, 233:1013-1017. PubMed Abstract | Publisher Full Text OpenURL

  44. Shimogori T, Banuchi V, Ng HY, Strauss JB, Grove EA: Embryonic signaling centers expressing BMP, WNT and FGF proteins interact to pattern the cerebral cortex.

    Development 2004, 131:5639-5647. PubMed Abstract | Publisher Full Text OpenURL

  45. Storm EE, Garel S, Borello U, Hebert JM, Martinez S, McConnell SK, Martin GR, Rubenstein JL: Dose-dependent functions of Fgf8 in regulating telencephalic patterning centers.

    Development 2006, 133:1831-1844. PubMed Abstract | Publisher Full Text OpenURL

  46. Monuki ES: The morphogen signaling network in forebrain development and holoprosencephaly.

    J Neuropathol Exp Neurol 2007, 66:566-575. PubMed Abstract | Publisher Full Text OpenURL

  47. Basson MA, Echevarria D, Ahn CP, Sudarov A, Joyner AL, Mason IJ, Martinez S, Martin GR: Specific regions within the embryonic midbrain and cerebellum require different levels of FGF signaling during development.

    Development 2008, 135:889-898. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  48. Selleck SB: Shedding light on the distinct functions of proteoglycans.

    Sci STKE 2006, 2006:pe17. PubMed Abstract | Publisher Full Text OpenURL

  49. Ornitz DM, Itoh N: Fibroblast growth factors.

    Genome Biol 2001, 2:REVIEWS3005. PubMed Abstract | BioMed Central Full Text | PubMed Central Full Text OpenURL

  50. DeHamer MK, Guevara JL, Hannon K, Olwin BB, Calof AL: Genesis of olfactory receptor neurons in vitro : regulation of progenitor cell divisions by fibroblast growth factors.

    Neuron 1994, 13:1083-1097. PubMed Abstract | Publisher Full Text OpenURL

  51. Gritti A, Frolichsthal-Schoeller P, Galli R, Parati EA, Cova L, Pagano SF, Bjornson CR, Vescovi AL: Epidermal and fibroblast growth factors behave as mitogenic regulators for a single multipotent stem cell-like population from the subventricular region of the adult mouse forebrain.

    J Neurosci 1999, 19:3287-3297. PubMed Abstract | Publisher Full Text OpenURL

  52. Vaccarino FM, Schwartz ML, Raballo R, Nilsen J, Rhee J, Zhou M, Doetschman T, Coffin JD, Wyland JJ, Hung YT: Changes in cerebral cortex size are governed by fibroblast growth factor during embryogenesis.

    Nat Neurosci 1999, 2:246-253. PubMed Abstract | Publisher Full Text OpenURL

  53. Maric D, Maric I, Chang YH, Barker JL: Prospective cell sorting of embryonic rat neural stem cells and neuronal and glial progenitors reveals selective effects of basic fibroblast growth factor and epidermal growth factor on self-renewal and differentiation.

    J Neurosci 2003, 23:240-251. PubMed Abstract | Publisher Full Text OpenURL

  54. Ohkubo Y, Uchida AO, Shin D, Partanen J, Vaccarino FM: Fibroblast growth factor receptor 1 is required for the proliferation of hippocampal progenitor cells and for hippocampal growth in mouse.

    J Neurosci 2004, 24:6057-6069. PubMed Abstract | Publisher Full Text OpenURL

  55. Zheng W, Nowakowski RS, Vaccarino FM: Fibroblast growth factor 2 is required for maintaining the neural stem cell pool in the mouse brain subventricular zone.

    Dev Neurosci 2004, 26:181-196. PubMed Abstract | Publisher Full Text OpenURL

  56. Kawauchi S, Shou J, Santos R, Hebert JM, McConnell SK, Mason I, Calof AL: Fgf8 expression defines a morphogenetic center required for olfactory neurogenesis and nasal cavity development in the mouse.

    Development 2005, 132:5211-5223. PubMed Abstract | Publisher Full Text OpenURL

  57. Maric D, Fiorio Pla A, Chang YH, Barker JL: Self-renewing and differentiating properties of cortical neural stem cells are selectively regulated by basic fibroblast growth factor (FGF) signaling via specific FGF receptors.

    J Neurosci 2007, 27:1836-1852. PubMed Abstract | Publisher Full Text OpenURL

  58. Saarimaki-Vire J, Peltopuro P, Lahti L, Naserke T, Blak AA, Vogt Weisenhorn DM, Yu K, Ornitz DM, Wurst W, Partanen J: Fibroblast growth factor receptors cooperate to regulate neural progenitor properties in the developing midbrain and hindbrain.

    J Neurosci 2007, 27:8581-8592. PubMed Abstract | Publisher Full Text OpenURL

  59. Thomson RE, Pellicano F, Iwata T: Fibroblast growth factor receptor 3 kinase domain mutation increases cortical progenitor proliferation via mitogen-activated protein kinase activation.

    J Neurochem 2007, 100:1565-1578. PubMed Abstract | Publisher Full Text OpenURL

  60. Linkhart TA, Clegg CH, Hauschka SD: Control of mouse myoblast commitment to terminal differentiation by mitogens.

    J Supramol Struct 1980, 14:483-498. PubMed Abstract | Publisher Full Text OpenURL

  61. Clegg CH, Linkhart TA, Olwin BB, Hauschka SD: Growth factor control of skeletal muscle differentiation: commitment to terminal differentiation occurs in G1 phase and is repressed by fibroblast growth factor.

    J Cell Biol 1987, 105:949-956. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  62. Mason I, Chambers D, Shamim H, Walshe J, Irving C: Regulation and function of FGF8 in patterning of midbrain and anterior hindbrain.

    Biochem Cell Biol 2000, 78:577-584. PubMed Abstract | Publisher Full Text OpenURL

  63. Chi CL, Martinez S, Wurst W, Martin GR: The isthmic organizer signal FGF8 is required for cell survival in the prospective midbrain and cerebellum.

    Development 2003, 130:2633-2644. PubMed Abstract | Publisher Full Text OpenURL

  64. Cholfin JA, Rubenstein JL: Frontal cortex subdivision patterning is coordinately regulated by Fgf8, Fgf17, and Emx2.

    J Comp Neurol 2008, 509:144-155. PubMed Abstract | Publisher Full Text OpenURL

  65. Xu J, Lawshe A, MacArthur CA, Ornitz DM: Genomic structure, mapping, activity and expression of fibroblast growth factor 17.

    Mech Dev 1999, 83:165-178. PubMed Abstract | Publisher Full Text OpenURL

  66. Xu J, Liu Z, Ornitz DM: Temporal and spatial gradients of Fgf8 and Fgf17 regulate proliferation and differentiation of midline cerebellar structures.

    Development 2000, 127:1833-1843. PubMed Abstract | Publisher Full Text OpenURL

  67. Liu A, Li JY, Bromleigh C, Lao Z, Niswander LA, Joyner AL: FGF17b and FGF18 have different midbrain regulatory properties from FGF8b or activated FGF receptors.

    Development 2003, 130:6175-6185. PubMed Abstract | Publisher Full Text OpenURL

  68. Galli A, Roure A, Zeller R, Dono R: Glypican 4 modulates FGF signalling and regulates dorsoventral forebrain patterning in Xenopus embryos.

    Development 2003, 130:4919-4929. PubMed Abstract | Publisher Full Text OpenURL

  69. Ford-Perriss M, Guimond SE, Greferath U, Kita M, Grobe K, Habuchi H, Kimata K, Esko JD, Murphy M, Turnbull JE: Variant heparan sulfates synthesized in developing mouse brain differentially regulate FGF signaling.

    Glycobiology 2002, 12:721-727. PubMed Abstract | Publisher Full Text OpenURL

  70. Kreuger J, Spillmann D, Li JP, Lindahl U: Interactions between heparan sulfate and proteins: the concept of specificity.

    J Cell Biol 2006, 174:323-327. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  71. Bishop JR, Schuksz M, Esko JD: Heparan sulphate proteoglycans fine-tune mammalian physiology.

    Nature 2007, 446:1030-1037. PubMed Abstract | Publisher Full Text OpenURL

  72. Song HH, Shi W, Xiang YY, Filmus J: The loss of glypican-3 induces alterations in Wnt signaling.

    J Biol Chem 2005, 280:2116-2125. PubMed Abstract | Publisher Full Text OpenURL

  73. Capurro MI, Xu P, Shi W, Li F, Jia A, Filmus J: Glypican-3 inhibits Hedgehog signaling during development by competing with patched for Hedgehog binding.

    Dev Cell 2008, 14:700-711. PubMed Abstract | Publisher Full Text OpenURL

  74. Fukuchi-Shimogori T, Grove EA: Neocortex patterning by the secreted signaling molecule FGF8.

    Science 2001, 294:1071-1074. PubMed Abstract | Publisher Full Text OpenURL

  75. Hebert JM, Mishina Y, McConnell SK: BMP signaling is required locally to pattern the dorsal telencephalic midline.

    Neuron 2002, 35:1029-1041. PubMed Abstract | Publisher Full Text OpenURL

  76. Hebert JM: Unraveling the molecular pathways that regulate early telencephalon development.

    Curr Top Dev Biol 2005, 69:17-37. PubMed Abstract | Publisher Full Text OpenURL

  77. Hebert JM, Fishell G: The genetics of early telencephalon patterning: some assembly required.

    Nat Rev Neurosci 2008, 9:678-685. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  78. Zhou CJ, Borello U, Rubenstein JL, Pleasure SJ: Neuronal production and precursor proliferation defects in the neocortex of mice with loss of function in the canonical Wnt signaling pathway.

    Neuroscience 2006, 142:1119-1131. PubMed Abstract | Publisher Full Text OpenURL

  79. Hayhurst M, Gore BB, Tessier-Lavigne M, McConnell SK: Ongoing sonic hedgehog signaling is required for dorsal midline formation in the developing forebrain.

    Dev Neurobiol 2008, 68:83-100. PubMed Abstract | Publisher Full Text OpenURL

  80. Hebert JM, Lin M, Partanen J, Rossant J, McConnell SK: FGF signaling through FGFR1 is required for olfactory bulb morphogenesis.

    Development 2003, 130:1101-1111. PubMed Abstract | Publisher Full Text OpenURL

  81. Garel S, Huffman KJ, Rubenstein JL: Molecular regionalization of the neocortex is disrupted in Fgf8 hypomorphic mutants.

    Development 2003, 130:1903-1914. PubMed Abstract | Publisher Full Text OpenURL

  82. Pan Y, Woodbury A, Esko JD, Grobe K, Zhang X: Heparan sulfate biosynthetic gene Ndst1 is required for FGF signaling in early lens development.

    Development 2006, 133:4933-4944. PubMed Abstract | Publisher Full Text OpenURL

  83. Grobe K, Inatani M, Pallerla SR, Castagnola J, Yamaguchi Y, Esko JD: Cerebral hypoplasia and craniofacial defects in mice lacking heparan sulfate Ndst1 gene function.

    Development 2005, 132:3777-3786. PubMed Abstract | Publisher Full Text OpenURL

  84. Williams RW, Herrup K: The control of neuron number.

    Annu Rev Neurosci 1988, 11:423-453. PubMed Abstract | Publisher Full Text OpenURL

  85. Oliver F, Christians JK, Liu X, Rhind S, Verma V, Davison C, Brown SD, Denny P, Keightley PD: Regulatory variation at glypican-3 underlies a major growth QTL in mice.

    PLoS Biol 2005, 3:e135. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  86. Chiao E, Fisher P, Crisponi L, Deiana M, Dragatsis I, Schlessinger D, Pilia G, Efstratiadis A: Overgrowth of a mouse model of the Simpson-Golabi-Behmel syndrome is independent of IGF signaling.

    Dev Biol 2002, 243:185-206. PubMed Abstract | Publisher Full Text OpenURL

  87. Crickmore MA, Mann RS: Hox control of morphogen mobility and organ development through regulation of glypican expression.

    Development 2007, 134:327-334. PubMed Abstract | Publisher Full Text OpenURL

  88. Baena-Lopez LA, Rodriguez I, Baonza A: The tumor suppressor genes dachsous and fat modulate different signalling pathways by regulating dally and dally-like.

    Proc Natl Acad Sci USA 2008, 105:9645-9650. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  89. Rawson JM, Dimitroff B, Johnson KG, Rawson JM, Ge X, Van Vactor D, Selleck SB: The heparan sulfate proteoglycans Dally-like and Syndecan have distinct functions in axon guidance and visual-system assembly in Drosophila.

    Curr Biol 2005, 15:833-838. PubMed Abstract | Publisher Full Text OpenURL

  90. Martin PT: Glycobiology of the synapse.

    Glycobiology 2002, 12:1R-7R. PubMed Abstract | Publisher Full Text OpenURL

  91. Yamaguchi Y: Glycobiology of the synapse: the role of glycans in the formation, maturation, and modulation of synapses.

    Biochim Biophys Acta 2002, 1573:369-376. PubMed Abstract | Publisher Full Text OpenURL

  92. Ethell IM, Yamaguchi Y: Cell surface heparan sulfate proteoglycan syndecan-2 induces the maturation of dendritic spines in rat hippocampal neurons.

    J Cell Biol 1999, 144:575-586. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  93. Johnson KG, Tenney AP, Ghose A, Duckworth AM, Higashi ME, Parfitt K, Marcu O, Heslip TR, Marsh JL, Schwarz TL, Flanagan JG, Van Vactor D: The HSPGs Syndecan and Dallylike bind the receptor phosphatase LAR and exert distinct effects on synaptic development.

    Neuron 2006, 49:517-531. PubMed Abstract | Publisher Full Text OpenURL

  94. Fukuhara N, Howitt JA, Hussain SA, Hohenester E: Structural and functional analysis of slit and heparin binding to immunoglobulin-like domains 1 and 2 of Drosophila Robo.

    J Biol Chem 2008, 283:16226-16234. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  95. Johnson KG, Ghose A, Epstein E, Lincecum J, O'Connor MB, Van Vactor D: Axonal heparan sulfate proteoglycans regulate the distribution and efficiency of the repellent slit during midline axon guidance.

    Curr Biol 2004, 14:499-504. PubMed Abstract | Publisher Full Text OpenURL

  96. Potkin SG, Turner JA, Guffanti G, Lakatos A, Fallon JH, Nguyen DD, Mathalon D, Ford J, Lauriello J, Macciardi F: A genome-wide association study of schizophrenia using brain activation as a quantitative phenotype.

    Schizophr Bull 2009, 35:96-108. PubMed Abstract | Publisher Full Text OpenURL

  97. O'Donovan MC, Norton N, Williams H, Peirce T, Moskvina V, Nikolov I, Hamshere M, Carroll L, Georgieva L, Dwyer S, Holmans P, Marchini JL, Spencer CC, Howie B, Leung HT, Giegling I, Hartmann AM, Möller HJ, Morris DW, Shi Y, Feng G, Hoffmann P, Propping P, Vasilescu C, Maier W, Rietschel M, Zammit S, Schumacher J, Quinn EM, Schulze TG, et al.: Analysis of 10 independent samples provides evidence for association between schizophrenia and a SNP flanking fibroblast growth factor receptor 2.

    Mol Psychiatry 2009, 14:30-36. PubMed Abstract | Publisher Full Text OpenURL

  98. Steen RG, Mull C, McClure R, Hamer RM, Lieberman JA: Brain volume in first-episode schizophrenia: systematic review and meta-analysis of magnetic resonance imaging studies.

    Br J Psychiatry 2006, 188:510-518. PubMed Abstract | Publisher Full Text OpenURL

  99. Ward KE, Friedman L, Wise A, Schulz SC: Meta-analysis of brain and cranial size in schizophrenia.

    Schizophr Res 1996, 22:197-213. PubMed Abstract | Publisher Full Text OpenURL

  100. Skarnes WC, Moss JE, Hurtley SM, Beddington RS: Capturing genes encoding membrane and secreted proteins important for mouse development.

    Proc Natl Acad Sci USA 1995, 92:6592-6596. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  101. Mitchell KJ, Pinson KI, Kelly OG, Brennan J, Zupicich J, Scherz P, Leighton PA, Goodrich LV, Lu X, Avery BJ, Tate P, Dill K, Pangilinan E, Wakenight P, Tessier-Lavigne M, Skarnes WC: Functional analysis of secreted and transmembrane proteins critical to mouse development.

    Nat Genet 2001, 28:241-249. PubMed Abstract | Publisher Full Text OpenURL

  102. Meyers EN, Lewandoski M, Martin GR: An Fgf8 mutant allelic series generated by Cre- and Flp-mediated recombination.

    Nat Genet 1998, 18:136-141. PubMed Abstract | Publisher Full Text OpenURL

  103. Maretto S, Cordenonsi M, Dupont S, Braghetta P, Broccoli V, Hassan AB, Volpin D, Bressan GM, Piccolo S: Mapping Wnt/beta-catenin signaling during mouse development and in colorectal tumors.

    Proc Natl Acad Sci USA 2003, 100:3299-3304. PubMed Abstract | Publisher Full Text | PubMed Central Full Text OpenURL

  104. Mombaerts P, Wang F, Dulac C, Chao SK, Nemes A, Mendelsohn M, Edmondson J, Axel R: Visualizing an olfactory sensory map.

    Cell 1996, 87:675-686. PubMed Abstract | Publisher Full Text OpenURL

  105. Wilkinson DG, Nieto MA: Detection of messenger RNA by in situ hybridization to tissue sections and whole mounts.

    Methods Enzymol 1993, 225:361-373. PubMed Abstract | Publisher Full Text OpenURL

  106. Zhang S, Lin Y, Itaranta P, Yagi A, Vainio S: Expression of Sprouty genes 1, 2 and 4 during mouse organogenesis.

    Mech Dev 2001, 109:367-370. PubMed Abstract | Publisher Full Text OpenURL

  107. Dickinson RJ, Eblaghie MC, Keyse SM, Morriss-Kay GM: Expression of the ERK-specific MAP kinase phosphatase PYST1/MKP3 in mouse embryos during morphogenesis and early organogenesis.

    Mech Dev 2002, 113:193-196. PubMed Abstract | Publisher Full Text OpenURL

  108. Goodrich LV, Johnson RL, Milenkovic L, McMahon JA, Scott MP: Conservation of the hedgehog/patched signaling pathway from flies to mice: induction of a mouse patched gene by Hedgehog.

    Genes Dev 1996, 10:301-312. PubMed Abstract | Publisher Full Text OpenURL

  109. Image J [http://rsb.info.nih.gov/ij/] webcite

  110. Cheng X, Hsu CM, Currle DS, Hu JS, Barkovich AJ, Monuki ES: Central roles of the roof plate in telencephalic development and holoprosencephaly.

    J Neurosci 2006, 26:7640-7649. PubMed Abstract | Publisher Full Text OpenURL

  111. Currle DS, Cheng X, Hsu CM, Monuki ES: Direct and indirect roles of central nervous system dorsal midline cells in choroid plexus epithelia formation.

    Development 2005, 132:3549-3559. PubMed Abstract | Publisher Full Text OpenURL

  112. Livak KJ, Schmittgen TD: Analysis of relative gene expression data using real-time quantitative PCR and the 2(-Delta Delta C(T)) Method.

    Methods 2001, 25:402-408. PubMed Abstract | Publisher Full Text OpenURL

  113. Walker JM: The bicinchoninic acid (BCA) assay for protein quantitation.

    Methods Mol Biol 1994, 32:5-8. PubMed Abstract OpenURL

  114. Herndon ME, Lander AD: A diverse set of developmentally regulated proteoglycans is expressed in the rat central nervous system.

    Neuron 1990, 4:949-961. PubMed Abstract | Publisher Full Text OpenURL