- Open Access
Ciliogenesis and cerebrospinal fluid flow in the developing Xenopus brain are regulated by foxj1
© Hagenlocher et al.; licensee BioMed Central Ltd. 2013
- Received: 6 May 2013
- Accepted: 3 September 2013
- Published: 24 September 2013
Circulation of cerebrospinal fluid (CSF) through the ventricular system is driven by motile cilia on ependymal cells of the brain. Disturbed ciliary motility induces the formation of hydrocephalus, a pathological accumulation of CSF resulting in ventricle dilatation and increased intracranial pressure. The mechanism by which loss of motile cilia causes hydrocephalus has not been elucidated. The aim of this study was: (1) to provide a detailed account of the development of ciliation in the brain of the African clawed frog Xenopus laevis; and (2) to analyze the relevance of ependymal cilia motility for CSF circulation and brain ventricle morphogenesis in Xenopus.
Gene expression analysis of foxj1, the bona fide marker for motile cilia, was used to identify potentially ciliated regions in the developing central nervous system (CNS) of the tadpole. Scanning electron microscopy (SEM) was used to reveal the distribution of mono- and multiciliated cells during successive stages of brain morphogenesis, which was functionally assessed by bead injection and video microscopy of ventricular CSF flow. An antisense morpholino oligonucleotide (MO)-mediated gene knock-down that targeted foxj1 in the CNS was applied to assess the role of motile cilia in the ventricles.
RNA transcripts of foxj1 in the CNS were found from neurula stages onwards. Following neural tube closure, foxj1 expression was seen in distinct ventricular regions such as the zona limitans intrathalamica (ZLI), subcommissural organ (SCO), floor plate, choroid plexus (CP), and rhombomere boundaries. In all areas, expression of foxj1 preceded the outgrowth of monocilia and the subsequent switch to multiciliated ependymal cells. Cilia were absent in foxj1 morphants, causing impaired CSF flow and fourth ventricle hydrocephalus in tadpole-stage embryos.
Motile ependymal cilia are important organelles in the Xenopus CNS, as they are essential for the circulation of CSF and maintenance of homeostatic fluid pressure. The Xenopus CNS ventricles might serve as a novel model system for the analysis of human ciliary genes whose deficiency cause hydrocephalus.
- Cerebrospinal fluid flow
- Choroid plexus
- Reissner’s fiber
- Subcommissural organ
- Zona limitans intrathalamica
Cerebrospinal fluid (CSF) is a clear liquid characterized by high ion and protein content that fills the ventricular system and subarachnoid space of the brain. Following neural tube closure, enlargement of the ventricles is driven by CSF secretion from ependymal cells. During later development, CSF is primarily secreted by the specialized epithelia of the highly vascularized choroid plexus (CP). CSF provides mechanical buffering to the brain, transports signaling molecules, and eliminates waste products from the ependyma . For this purpose, CSF generated inside the ventricles has to be actively transported through the system of lateral, third, and fourth ventricles into the subarachnoid space, where it is reabsorbed into the venous system .
In patients suffering from hydrocephalus this process is disturbed, resulting in increased intra-ventricular pressure, enlargement of the lumina, and damage to brain tissue. Hydrocephalus may result from an overproduction of CSF, impaired reabsorption or by obstruction of any of the ventricular ducts and foramina, that is, the narrow passageways through which CSF flows from one ventricle to the next as well as into the subarachnoid space . Obstructions may be caused by hemorrhage, tumors, or morphogenetic malformations of ventricle-contacting tissues . Immotile cilia result in impaired CSF transport (ependymal flow) as well, as encountered in certain ciliopathies [4, 5]. Ciliary immotility leading to hydrocephalus has been shown to result from mutations in structural proteins, such as Spag6  or axonemal motor proteins such as Dnahc5. Mice deficient in Mdnah5 for example have no detectable ependymal flow, ultimately leading to stenosis of the cerebral aqueduct and hydrocephalus in the lateral and third ventricles [5, 7]. On the regulatory level, transcription factors of the regulatory factor X (RFX) and winged-helix (forkhead, FOX) families govern the differentiation of cells towards a ciliated phenotype. RFX3-deficiency leads to aberrant ciliation and hydrocephalus in mice . The winged-helix family member foxj1 acts as a master regulator of genes inducing the biogenesis of motile cilia . In zebrafish and mouse, loss of Foxj1 function leads to a loss of motile, but not immotile cilia [9–12], and Foxj1 knock-out mice develop hydrocephalus postnatally [10, 11]. Transcription of Foxj1 marks the onset of ciliogenesis in all embryonic tissues studied so far, rendering Foxj1 a bona fide marker gene for motile cilia .
The present study provides a detailed account of the development of motile cilia in the Xenopus tadpole brain, up to the onset of metamorphosis. Cilia-driven CSF flow was assessed by video microscopy following injection of fluorescent microspheres into the ventricles. CSF flow was compromised in foxj1 morphants, which developed hydrocephalus at tadpole stage. Our study provides an entry point into using Xenopus as a model system for studying human ciliary genes whose deficiency cause hydrocephalus.
All animals were treated according to the German regulations and laws for care and handling of research animals, and experimental manipulations according to § 6, article 1, sentence 2, No. 4 of the Animal Protection Act were approved by the Regional Government Stuttgart, Germany (Vorhaben A 365/10 ZO ‘Molekulare Embryologie’).
RNA in situhybridization and histological analysis
Embryos were fixed for 2 h in 1 × MEMFA consisting of one part of 10 × MEMFA (1 M MOPS, pH 7.4, Roth; 20 mM EGTA; 10 mM MgSO4, both Applichem), one part formaldehyde (37%, Roth) and eight parts H2O. Where indicated, larval brains were explanted and embryos as well as explants were processed following standard protocols . A digoxigenin (Roche)-labeled RNA probe was prepared from linearized plasmid containing the full-length sequence of foxj1 using T7 RNA polymerase (Promega). In situ hybridization was performed according to . For histological analysis embryos were embedded in gelatin-albumin and sectioned on a vibratome at 30 to 40 μm.
For scanning electron microscope (SEM) analyses, brains were explanted, bisected, further processed as described  and viewed at 10 kV on a Jeol SEM.
MO-mediated knock-down of foxj1
One pmol of foxj1 antisense morpholino oligonucleotide (MO, Gene Tools, Philomath, OR, USA) was injected into the animal region of each dorsal blastomere of four to eight cell-stage embryos using a Harvard Apparatus setup. The foxj1MO targeted the initiation codon as described in . Dextran tetramethylrhodamine (MW 70.000, 0.5-1 μg/μL, Invitrogen) was used as a lineage tracer. In all experiments, care was taken to exclusively use embryos with a clear dorsoventral segregation of pigment , and only correctly targeted specimens (controlled by lineage tracer fluorescence in the CNS at stage 21) were processed for further analysis.
Measurement of ventricles
CSF flow analysis
Embryos were anesthetized using benzocaine (E1501, Sigma). Fluorescent microbeads (F8823, FluoSpheres® carboxylate-modified microspheres, 1.0 μm, yellow-green fluorescence (505/515), 2% solids, Invitrogen, Molecular Probes) were diluted 1/250 into a solution of 0.5-1 μg/μL dextran tetramethylrhodamine in 1 × MBSH. A volume of about 20 nL was injected into the fourth ventricle using a pulled-out glass micropipette. Glass pipettes (Hilgenberg) were prepared using a Sutter Instruments Flaming/Brown micropipette puller (P-87; heat 720, pull 30, velocity 290, time 3) to yield pipettes with a short taper and short tip for enhanced stability. Embryos were embedded in 1 × MBSH buffer. The coverslip was adjusted in height using vaseline as a flexible spacer. Movement of beads was documented on a Zeiss Axioskop 2 (Zeiss) using a 20 × Plan-Neofluar objective (Zeiss) by taking 1,000 frame-long time-lapse movies at 175 fps using a Zeiss Axiocam HSm (size of region of interest, ROI, 660 × 128 px) and Axiovision 4.7 together with the ‘fast recorder’ plug-in.
To visualize the directionality of moving beads, 20 consecutive raw frames were color-coded from red to green (green representing the current position of the particle) and projected onto a single frame by using a custom interpretation of the ‘Temporal-Color Coder’ (Kota Miura, EMBL, Heidelberg) plug-in for Fiji . Particle movement was analyzed towards velocity of single beads using the ImageJ plug-in ParticleTracker [18, 20], which saves the coordinates of the trajectories. All trajectories matching the analysis criteria were then further processed with the help of a custom-made program written in statistical R (The R project for statistical computing; http://www.r-project.org/) which calculated the length and velocity of each particle track .
P values were calculated using the Mann–Whitney U-test in statistical R. In order to account for multiple testing, P values are reported after strict bonferroni correction at nominal levels * <0.05, ** <0.01, and *** <0.001 (adjusted levels * <0.0166, ** <0.0033, *** <0.00033 for n = 3).
Xenopus tadpoles express foxj1in distinct regions of the developing CNS
During cephalic ventricle inflation and flexion (stage 25), a bilateral foxj1 domain was seen in the minor groove of the cephalic flexure (arrowhead in Figure 1D”), which represents the rostral continuation of the spinal cord and rhombencephalic floor plate. This prosencephalic expression persisted through stage 36 (arrowheads in Figure 1E”, F”). When stage 36 brain explants were probed for foxj1 (Figure 1G) or shh (Figure 1H) expression, respectively, domains were found to overlap, identifying the foxj1-positive area in the future diencephalon as the zona limitans intrathalamica (ZLI; ). The ZLI represents an important signaling center for diencephalon development .
Continued foxj1expression correlates with elongation of monocilia and the emergence of multiciliation
In order to investigate whether sites of foxj1 expression correlated with cilia formation, whole-mount explants of brains were analyzed in parallel by scanning electron microscopy (SEM). The first stage for which brains could be successfully explanted was stage 35. Earlier specimens frequently ruptured due to the high content of yolk, which was consumed around stage 35. foxj1 continued to be expressed in the floor plate, ZLI and SCO at that stage (Figure 2A). Brains cut sagittally along the midline and prepared for SEM analysis revealed the internal organization of the ventricular surface; pros-, mes-, and rhombencephalon could be easily distinguished (Figure 2B). The rostral part of the prosencephalon was strongly bent downward and brains measured about 1 mm in length (measured as a straight line from the rostral-most extension of the prosencephalon to the rhombencephalon/spinal cord transition; Figure 2B). A furrow developing in the preoptic region was visible as well, which delineated the developing boundary between tel- and diencephalon as well as the epiphysis (pineal gland) on the dorsal roof of the posterior prosencephalon (Figure 2B). The ZLI was obvious as a V-shaped wedge of tissue in the posterior prosencephalon. The metameric organization of the rhombencephalon was easily discernible by the boundaries between the rhombomeres which appeared as vertical slit-like structures (Figure 2B).
The ependymal surface of stage 35 brains was predominantly constituted by cells which harbored short monocilia (1–2 μm; Figure 2C, D; arrowheads in Figure 2C’, D’). In addition, cells with single elongated cilia were identified (4–6 μm; Figure 2C, D; outlined arrowheads in Figure 2C”, D”, E), as well as first oligociliated cells (red arrowhead in Figure 2E). The localization of ciliated cells correlated with preceding expression of foxj1, as cells with elongated monocilia appeared in the ZLI (Figure 2C) as well as in the rhombencephalic ventral midline (Figure 2D). Cells of the rhombencephalon roof also harbored elongated monocilia, where several oligociliated cells were intermingled as well (Figure 2E).
At stage 40, foxj1 expression was found generally unchanged in brains of comparable morphology (Additional file 1: Figure S1A, B). The brain had begun to straighten, a process which continued through stage 43. Brain length at stage 40 still was about the same as at stage 35. Tel-, di-, mes-, and rhombencephalon were easily distinguishable (Additional file 1: Figure S1A, B). While primary cilia in most brain regions remained short (1–2 μm, Additional file 1: Figure S1C, D; arrowheads in Additional file 1: Figure S1C’, D’), elongated cilia continued to appear and reached maximum lengths of about 9 μm (Additional file 1: Figure S1C, D; outlined arrowheads in Additional file 1: Figure S1C”, D”). The rhombencephalic roof showed multiciliated cells (MCCs) with cilia of 4–5 μm in length (arrowhead in Additional file 1: Figure S1E). Around stage 45, the pattern of foxj1 expression in the brain was supplemented by two additional domains - one spot just anterior to the SCO in the telencephalon (outlined arrowhead in Figure 3A) and a striped pattern in the rhombencephalon (Figure 3A). The completely straightened brain still measured about 1 mm in length and was entirely surrounded by the dura mater. The ventricle underlying the optic tectum widened and invagination of the third ventricle CP began (Figure 3B).
Histological vibratome sections of in situ-hybridized brains were used for more detailed correlation of foxj1 expression and ciliation patterns. Transverse sections through the anterior spot-shaped expression domain of foxj1 revealed staining in the developing CP of the lateral/third ventricles (Figure 3A’). The CP starts to grow and invaginate into the ventricular system at stage 43 . It became visible as a thickened indentation of the dorsal roof at the tel-/diencephalon junction by SEM, and its ventricular surface was covered densely with MCCs (Figure 3C). In sections at the level of the di-/mesencephalic boundary, staining in both the SCO and ZLI was apparent (Figure 3A”). In the SCO, SEM pictures revealed elongated cilia, to which uncharacterized extracellular material was attached (Figure 3D). The SCO generates Reissner’s fiber (RF), which is composed of aggregated glycoproteins such as SCO-spondin. The RF forms a thread which runs through the entire ventricular system and central canal of the spinal cord . The material sticking to SCO cilia perhaps reflected the production of RF in Xenopus, which we frequently witnessed spanning the ventricular lumen (not shown; cf. Figure 4F). The ventricular surface area corresponding to sites of foxj1 expression found in the ZLI in transverse sections consisted of cells with elongated monocilia, comparable to those seen in the ZLI in stage 35/40 embryos (Figure 3D).
Higher magnification of the ventricular surface of the rhombencephalon in dissected brains (Figure 3A) as well as in transverse sections (Figure 3A’”, A””) identified the striped pattern on the lateral walls of the fourth ventricle as the metameric organization of the rhombencephalon. While cells located at the center of the rhombomeres were free of foxj1 expression (rh; Figure 3A’”), transcripts were found in cells at the rhombomere boundaries (rhb; Figure 3A””). This expression pattern was reflected by a differential organization of cilia. Cells with short monocilia covered the foxj1-negative regions of the rhombomeres (Figure 3E and arrowheads in E’), whereas the foxj1-positive cells at the boundaries of the rhombomeres carried monocilia of 9–10 μm length (Figure 3E, E”).
Similar to the lateral/third ventricles, the roof of the fourth ventricle starts to thicken and a highly vascularized CP epithelium forms around stage 43 . Cross-sections through the fourth ventricle CP at stage 45 showed strong expression of foxj1 (Figure 3A’”, A””) and SEM revealed the presence of multiciliary tufts on the surface of fourth ventricle CP cells (Figure 3F, G). By stage 53, foxj1 expression had become very pronounced, extending to all ventricle-lining epithelia (Figure 4A). Brains measured about 2 mm in length and all parts were well developed (Figure 4B). Staining in the medial and lateral domains of the CP at the boundary between the lateral and third ventricle intensified considerably over time, concomitant with the growth and vascularization of the CP tissue, which protruded into the ventricular lumen at stage 53 (Figure 4A’). SEM revealed the highly convoluted arrangement of blood vessels covered with MCCs (Figure 4C).
Sections running through the di-/mesencephalic boundary showed a continually strong expression of foxj1 in the SCO and ZLI. Additionally, foxj1 started to be expressed in the ventricular layer of the fully developed pituitary (hypophysis (hy); Figure 4A”). The continuous expression of foxj1 in the SCO and ZLI was reflected by the morphological development of cilia in these regions. Cilia in the SCO were elongated, however, whether cells of the SCO were mono- or multiciliated could not be discerned (Figure 4D). In the ZLI and at the di-/mesencephalic boundary, the first multiciliary tufts became apparent on the surface of cells (Figure 4E). Corresponding to the onset of foxj1 expression, luminal cells of the neurohypophyseal infundibulum bore elongated monocilia and in several cases, multiciliary tufts were visible on cells of the infundibular roof (Additional file 2: Figure S2).
In the cerebral aqueduct (CA), cells were studded with elongated monocilia and RF frequently spanned the aqueduct lumen (Figure 4F). Similar to all other ventral regions of the stage 53 brain, the ventral midline of the rhombencephalon was covered with long mono- and multicilia (Figure 4G). The striped expression of foxj1 in the rhombencephalon (Figure 4A, A’”, A””) and the corresponding ciliation pattern was still obvious. While monocilia at the center of rhombomeres remained short, cilia in the boundary regions elongated further and the boundary domain appeared wider (Figure 4H). Similar to the development of the lateral/third ventricle CP, the CP of the rhombencephalon roof developed into an elaborate convoluted structure, the surface of which was covered with MCCs (Figure 4I). In the adult brain, ventricle-contacting cells had developed into a single-layered ependymal epithelium which became apparent in areas, in which the continuous layer had been disrupted during fixation and processing of specimens (arrowheads in Figure 4J, K). Close-up views revealed that the adult ependyma consisted of MCCs throughout (Figure 4L).
Taken together, neural expression of foxj1 correlated with ciliation patterns in Xenopus tadpole brains, such that the first elongated cilia arose in regions of early foxj1 expression. Sustained transcription in these and additional regions mirrored the continuous development from short to elongated monocilia, eventually resulting in multiciliation of the entire brain ependyma.
foxj1loss of function induces hydrocephalus
CSF flow analysis following injection of both dye solution and microbeads revealed even distribution throughout the ventricular system of control embryos (Figure 5D). However, fluorescent signals were frequently absent from the forebrain of foxj1 morphant specimens (Figure 5E). In the few cases when dye penetrated into the forebrain, ventricles appeared severely misshapen (Additional file 3: Figure S3). Hindbrain ventricles, however, were always completely filled with dye and markedly inflated in foxj1 morphants (Figure 5E; Additional file 3: Figure S3). Hydrocephalic expansion of the fourth ventricle was quantitatively assessed by calculating the width-to-length ratio in control and foxj1MO-injected embryos (red arrows in Figure 5D). Compared to either control type, in which the fourth ventricle appeared elliptical, the ventricle shape of foxj1 morphants was shifted towards a more circular appearance (Figure 5H; P = 0.00191 and P = 0.001541).
Additional file 4: Movie S5. CSF flow in the fourth ventricle. Movie illustrating patterns of cerebrospinal fluid flow in the fourth ventricle of an untreated control embryo at stage 46 upon injection of fluorescent microbeads. Focus plane of the movie shifts in five steps from dorsal (d) to ventral (v) as indicated by the red line in the schematic cross section through the fourth ventricle presented in the inset. Every frame of the movie comprises 20 consecutive raw frames that were color-coded from red to green and projected onto a single frame by using a custom interpretation of the "Temporal-Color Coder" (Kota Miura, EMBL, Heidelberg) plug-in for Fiji. Note the fast rostrally-directed flow just underneath the dorsal roof, change of flow direction in medial focus planes, and caudally-directed flow in the ventral-most focus planes. Movie plays in real time. a = anterior; p = posterior. (MOV 9 MB)
In order to image cilia-driven flow without the influence of the dorsal MCCs of the rhombencephalon roof, brains were excised and dissected along the dorsal midline to remove the dorsal roof. Explants were flat-mounted in fluid-filled chambers, which contained beads to image flow on the ventral and lateral ventricular surface of the fourth ventricle. Fluid flow driven by motile cilia was detected both medially along the ventral midline as well as lateral to the midline. Lateral flow was linear from rostral to caudal, however, it was interrupted and re-initiated by the motile cilia at the rhombomere boundaries (Additional file 5: Movie S6). Analyses of CSF flow thus strongly suggested that all elongated cilia in the rhombencephalon, including the monocilia at the rhombomere boundaries, were motile and produced fluid flow. The data also demonstrated that multiciliated CP cells were the driving force of CSF flow, which are necessary and sufficient to generate the circulatory movement of fluid detected in the fourth ventricle.
For a detailed analysis of CSF flow parameters, regions of interest were chosen at the center of the ventricle (blue box in Figure 5E) and the focus plane was adjusted such that laminar flow driven by ciliary bundles on the dorsal roof was recorded (refer to Figure 3F, G). Beads were rapidly propelled in a caudal to rostral fashion; bead movement was visualized by maximum z-projection of the time series and trajectories computed by the ImageJ plug-in ParticleTracker (Figure 5F’, G’; Additional file 6: Movie S7). Comparison of trajectories from control and foxj1 morphant specimens revealed three prominent features: (1) CSF flow was severely impaired in morphants; (2) the degree with which cilia were lost on cells of the rhombencephalon roof varied. In some patches beads were still propelled in a directed manner (red asterisk in Figure 5G), whereas no moving beads were detected in between these patches (yellow asterisk in Figure 5G), indicating that in such areas cells had lost motile cilia altogether; (3) bead velocities were compromised in morphants (Figure 5I). In uninjected control embryos, the mean velocities were determined at 401 ± 100 μm/s. coMO-injected specimens ranged at around an average of 439 ± 86 μm/s, a deviation that was not statistically significant (P = 0.4557). foxj1 morphants, in contrast, showed a significant reduction of bead velocities with 235 ± 96 μm/s (P = 0.0011 morphant vs. uninjected; P = 0.00022 morphant vs. coMO). When ventricle shape (Figure 5H) of individual embryos was plotted against flow velocity (refer to Figure 5I), the shape of ventricles was consistently elliptical within the control group (Figure 5J), even though flow velocities in control specimens varied between 300–600 μm/s. In foxj1 morphants, CSF flow velocity dropped to <300 μm/s which strongly correlated with a bias towards a rounded appearance of the ventricle, that is, hydrocephalic inflation. In summary, loss of foxj1 in the Xenopus CNS resulted in hydrocephalus of the fourth ventricle and a significant decrease in CSF flow velocity.
CSF flow velocity is caused by motile cilia
In summary, our analyses revealed a critical role of foxj1 for motile cilia and CSF flow in the developing Xenopus brain. Our data underscore the function of CSF flow for brain morphogenesis and establish a connection between impaired ciliary motility and hydrocephalus.
Expression of foxj1precedes and is spatially correlated with the emergence of elongated cilia
During vertebrate embryonic development, all neuroepithelial and radial glia cells initially carry an immotile monocilium on their apical surface which faces the ventricular lumen . In the mouse, differentiation of the ventricle-lining ependyma into a single layer of cuboidal MCCs occurs towards the end of the first postnatal week . Neural expression of Foxj1 precedes the emergence of ependymal cilia, as transcripts were detected during mouse embryonic development. Sites of Foxj1 transcription during mouse neurulation (embryonic day E10/13.5) include the rostral-most rhombomeres, mid-/hindbrain boundary, caudal midline, mesencephalic vesicle, ventro-lateral forebrain and CPs of the lateral, third, and fourth ventricles [12, 35]. Foxj1 is thus expressed in homologous regions during embryogenesis of mouse and frog. If one considers the onset of metamorphosis in amphibians roughly equivalent to birth in mammals, also the time course of Foxj1 expression in the mouse brain complies with our observations in the Xenopus brain. Preceding the general appearance of ependymal cilia in the mouse, MCCs have been identified in the epithelia of the mesencephalic cerebral aqueduct as well as the CP at postnatal day (P) 1 . Beyond CP and aqueduct we identified additional sites of ciliation in the Xenopus tadpole brain, in particular in the SCO, ZLI, and ventro-lateral rhombencephalon, all of which expressed foxj1 prior to the elongation of cilia. It will be interesting to analyze whether the foxj1/cilia module at these sites is conserved in the mouse as well.
Transcription factors of the RFX family governing ciliogenesis are also expressed in neural tissue during Xenopus embryonic development . However, while RFX family members 1–5 are found throughout the sensorial layer during neural fold apposition and closure, foxj1 is restricted to the ventral midline and floor plate at the same stages. This illustrates that RFX factors and foxj1 have overlapping yet distinct functions in ciliogenesis. While RFX factors in neural tissue seem to be required for both the primary cilia of sensorial layer cells and the prospective motile cilia of the floor plate, foxj1 acts as the master regulator for motile cilia.
Interestingly, during late embryogenesis (stage 45/46), when vigorous and rapid CSF flow has developed, only a few areas of the brain expressing foxj1 were multiciliated, while the remainder of foxj1-expressing cells harbored elongated monocilia. Multiciliation developed later in areas with sustained foxj1 expression. This observation is in perfect agreement with the notion that low levels of foxj1 expression induce cells to form an elongated motile monocilium . The switch of a cell’s ciliation from an elongated motile monocilium to multiple motile cilia requires expression of the small coiled-coil domain-containing protein multicilin . Based on the time points of MCC emergence identified here, it will be interesting to analyze the appearance of multicilin expression in the Xenopus brain.
CSF flow is driven by motile cilia
Two recent studies have described CSF flow patterns in the Xenopus tadpole brain [32, 38]. Motile cilia were proposed as a possible cause, based on reports of ciliated ventricles in other anuran species [39, 40]. Heartbeat was discussed as an alternative or additional mode of CSF flow control, as anesthesia of tadpoles with MS-222, which resulted in slowed or absent heartbeat, reduced flow velocities from 77 μm/s to 11 μm/s . MS-222 is known to acidify aqueous solutions, and low pH in turn reduces ciliary beat frequency (CBF) . We used benzocaine as an anesthetic and our experimental setup was designed to limit dose (<0.01%) and incubation time prior to bead injection (<5′) as much as possible, which might explain why we have not encountered heartbeat-dependence of CSF flow. The overall much higher CSF flow velocities in our study (450 μm/s) might be explained through avoidance of unspecific effects on pH and CBF as well. Taken together our data strongly suggest that cilia are the sole source of CSF flow in Xenopus, notwithstanding the role of blood flow in maintaining the physiological function of the CP.
Absence of motile cilia causes hydrocephalus
Even though mutations in cilia-associated genes are well-documented in the etiology of hydrocephalus [42, 43], the mechanism of how a loss of motile cilia causes hydrocephalic inflation of the ventricles has remained unclear. Since the loss of motile cilia in foxj1 morphants affects diverse cell populations in the developing brain it is conceivable that the development of hydrocephalus might be multifactorial.
In our foxj1 gene knock-down experiments, cilia in the Xenopus ventricles were not entirely absent. Consequently, flow was never completely abolished, although velocities were significantly reduced. Remarkably, a drop below a critical threshold of 300 μm/s was correlated with fourth ventricle hydrocephalus in individual morphant tadpoles. The rostrally directed CSF flow at the roof of the rhombencephalon presents the most vigorous one of the entire ventricular system (450 μm/s vs. 160 μm/s at the anterior CP). Flow rates <300 μm/s might fail to create enough pressure to force CSF through the aqueduct into the forebrain ventricles. It is tempting to speculate that this failure of CSF penetration into the forebrain could result in a secondary effect - a collapse of forebrain ventricles, which we have frequently witnessed in foxj1 morphant brains (Additional file 3: Figure S3).
A collapse of the forebrain ventricles or stenosis of the mesencephalic aqueduct might alternatively result from foxj1 loss of function in the fore-/midbrain area. Aqueduct stenosis preceding the occurrence of hydrocephalus has been described in rats in which the formation of RF by the SCO was manipulated . This notion was recently supported by an analysis of rats with morphological and functional deficiency of the SCO . RF is thought to keep the aqueduct open, and manipulations interfering with secretion or aggregation of RF-glycoproteins lead to collapse of the aqueduct and subsequent hydrocephalus in late postnatal stages. In Xenopus, Reissner’s substance (the RF precursor) is first produced by cells of the floor plate and subsequently by the developing SCO . Both floor plate and SCO are regions with prominent foxj1 expression and ciliation in the SCO has been severely affected in our foxj1 knock-down experiments (Figure 6). The loss of motile cilia through depletion of foxj1 might affect the production and/or distribution of RF, causing aberrant ventricular morphology in the fore- and midbrain and in the end hydrocephalus of the hindbrain. Aqueduct stenosis has also been described as the cause of hydrocephalus occurring postnatally in mice deficient for Mdnah5, which show loss of ciliary motility on ependymal cells .
However, hydrocephalus can also occur independently of aqueduct stenosis as seen in RFX3-deficient mice . Here, loss of RFX3 causes aberrant ciliation in the SCO and a decrease in RF immunoreactivity, leading to congenital hydrocephalus without collapse of the aqueduct. Even though SCO ciliation is altered in RFX3 mice, ependymal cilia are motile. It thus seems plausible that the correct inflation and shape of the ventricular system is determined by an interplay of ciliary motility, developmental RF production, and postnatal SCO function. Variations in these factors might determine some of the morphological differences. Future analyses will evaluate to what degree loss of function of foxj1 causes perturbations in the SCO and impairment of RF production.
Another possible origin of hydrocephalus might be an overproduction of CSF, leading to increased fluid pressure in the ventricular system. In the mouse, dysfunctional cilia on the CP have been implicated in the misregulation of CSF production . As the entire roof of the Xenopus rhombencephalon constitutes a CSF-secreting CP, which was impaired in foxj1 morphants, it is conceivable that an altered secretory activity of CP cells may have led to an overproduction of CSF as well.
Remarkably, foxj1 knock-down led to conspicuous morphogenetic changes in the di-/mesencephalon as well, reflected by a shortening of the affected area along the rostro-caudal axis. The affected area harbors the ZLI, an important signaling center for thalamus determination during embryonic brain development. Other signaling centers in the embryonic CNS comprise the floor plate, the isthmus (mid/hindbrain) organizer, and the rhombomere boundaries. Interestingly, rhombomere boundary cells expressed foxj1 and had a single elongated motile cilium on their surface. Although the functional significance of this correlation remains elusive, it is well established that rhombomere boundary cells serve as signaling centers, involved in the maintenance of the metameric identity of the hindbrain [47–49]. A defining characteristic of all the aforementioned signaling centers seems to be that they express foxj1 and develop single elongated motile cilia (Additional file 7: Figure S4). These cilia may play a pivotal role for the functionality of these signaling centers, through propagation of morphogen gradients and/or detecting and processing signaling molecules. The patterning of the rhombencephalon is governed by three signaling centers (floor plate, rhombomere boundaries, and isthmus organizer). The loss of motile cilia in each of these centers in foxj1 morphants may thus disturb hindbrain morphogen gradients, and together with reduced flow velocity and aqueduct stenosis cause hydrocephalic enlargement of the fourth ventricle. Taken together, the absence of motile cilia may impact on a multitude of processes in diverse parts of the brain, some or a combination of which may result in the development of hydrocephalus.
Hydrocephalus presents a common birth defect in humans, occurring with a frequency of 0.1-0.3% of live births . Among other causes, congenital hydrocephalus has been attributed to a loss of ciliary motility in the brain ventricles and the consequential loss of CSF movement. The Xenopus tadpole brain constitutes an attractive novel model system to study the formation of hydrocephalus during embryogenesis. The present study provides a reference point with its precise account of the temporal-spatial appearance of motile mono- and multiciliated cells and the assessment of CSF flow in live specimens. Morphant tadpoles deficient in foxj1, which lack motile cilia and consequently develop hydrocephalus, demonstrate the general validity of the system. Emerging new techniques for gene knock-down and allele replacement in Xenopus should offer an opportunity to directly analyze the role of human genes whose deficiency may cause hydrocephalus formation.
We thank Martin Blum for support and critical reading of the manuscript, Anna Iwanska for expert technical help, and members of the Blum lab for discussion. CH and KF are indebted to the Baden-Württemberg Stiftung for the financial support of this research project by the Eliteprogramme for Postdocs. PW was a recipient of a PhD fellowship from the Landesgraduiertenförderung, TT received a Heidelberg CellNetworks Cluster of Excellence postdoctoral fellowship, and KF was supported by a Margarete-von-Wrangell fellowship, funded by the European Social Fund and by the Ministry Of Science, Research and the Arts in Baden-Württemberg.
- Brown PD, Davies SL, Speake T, Millar ID: Molecular mechanisms of cerebrospinal fluid production. Neuroscience. 2004, 129: 957-970.View ArticlePubMedPubMed CentralGoogle Scholar
- Kapoor KG, Katz SE, Grzybowski DM, Lubow M: Cerebrospinal fluid outflow: an evolving perspective. Brain Res Bull. 2008, 77: 327-334. 10.1016/j.brainresbull.2008.08.009.View ArticlePubMedGoogle Scholar
- Del Bigio MR: Ependymal cells: biology and pathology. Acta Neuropathol. 2010, 119: 55-73. 10.1007/s00401-009-0624-y.View ArticlePubMedGoogle Scholar
- Sawamoto K, Wichterle H, Gonzalez-Perez O, Cholfin J, Yamada M, Spassky N, Murcia N, Garcia-Verdugo J, Marin O, Rubenstein J, Tessier-Lavigne M, Okano H, Alvarez-Buylla A: New neurons follow the flow of cerebrospinal fluid in the adult brain. Science. 2006, 311: 629-632. 10.1126/science.1119133.View ArticlePubMedGoogle Scholar
- Ibañez-Tallon I, Pagenstecher A, Fliegauf M, Olbrich H, Kispert A, Ketelsen UP, North A, Heintz N, Omran H: Dysfunction of axonemal dynein heavy chain Mdnah5 inhibits ependymal flow and reveals a novel mechanism for hydrocephalus formation. Hum Mol Genet. 2004, 13: 2133-2141. 10.1093/hmg/ddh219.View ArticlePubMedGoogle Scholar
- Sapiro R, Kostetskii I, Olds-Clarke P, Gerton GL, Radice GL, Strauss JF: Male infertility, impaired sperm motility, and hydrocephalus in mice deficient in sperm-associated antigen 6. Mol Cell Biol. 2002, 22: 6298-6305. 10.1128/MCB.22.17.6298-6305.2002.View ArticlePubMedPubMed CentralGoogle Scholar
- Ibañez-Tallon I, Gorokhova S, Heintz N: Loss of function of axonemal dynein Mdnah5 causes primary ciliary dyskinesia and hydrocephalus. Hum Mol Genet. 2002, 11: 715-721. 10.1093/hmg/11.6.715.View ArticlePubMedGoogle Scholar
- Baas D, Meiniel A, Benadiba C, Bonnafe E, Meiniel O, Reith W, Durand B: A deficiency in RFX3 causes hydrocephalus associated with abnormal differentiation of ependymal cells. Eur J Neurosci. 2006, 24: 1020-1030. 10.1111/j.1460-9568.2006.05002.x.View ArticlePubMedGoogle Scholar
- Yu X, Ng CP, Habacher H, Roy S: Foxj1 transcription factors are master regulators of the motile ciliogenic program. Nat Genet. 2008, 40: 1445-1453. 10.1038/ng.263.View ArticlePubMedGoogle Scholar
- Brody SL, Yan XH, Wuerffel MK, Song SK, Shapiro SD: Ciliogenesis and left-right axis defects in forkhead factor HFH-4-null mice. Am J Respir Cell Mol Biol. 2000, 23: 45-51. 10.1165/ajrcmb.23.1.4070.View ArticlePubMedGoogle Scholar
- Chen J, Knowles HJ, Hebert JL, Hackett BP: Mutation of the mouse hepatocyte nuclear factor/forkhead homologue 4 gene results in an absence of cilia and random left-right asymmetry. J Clin Invest. 1998, 102: 1077-1082. 10.1172/JCI4786.View ArticlePubMedPubMed CentralGoogle Scholar
- Jacquet BV, Salinas-Mondragon R, Liang H, Therit B, Buie JD, Dykstra M, Campbell K, Ostrowski LE, Brody SL, Ghashghaei HT: FoxJ1-dependent gene expression is required for differentiation of radial glia into ependymal cells and a subset of astrocytes in the postnatal brain. Development. 2009, 136: 4021-4031. 10.1242/dev.041129.View ArticlePubMedPubMed CentralGoogle Scholar
- Vick P, Schweickert A, Weber T, Eberhardt M, Mencl S, Shcherbakov D, Beyer T, Blum M: Flow on the right side of the gastrocoel roof plate is dispensable for symmetry breakage in the frog Xenopus laevis. Dev Biol. 2009, 331: 281-291. 10.1016/j.ydbio.2009.05.547.View ArticlePubMedGoogle Scholar
- Stubbs JL, Oishi I: Izpisúa Belmonte JC, Kintner C: The forkhead protein Foxj1 specifies node-like cilia in Xenopus and zebrafish embryos. Nat Genet. 2008, 40: 1454-1460. 10.1038/ng.267.View ArticlePubMedPubMed CentralGoogle Scholar
- Belo JA, Bouwmeester T, Leyns L, Kertesz N, Gallo M, Follettie M, De Robertis EM: Cerberus-like is a secreted factor with neutralizing activity expressed in the anterior primitive endoderm of the mouse gastrula. Mech Dev. 1997, 68: 45-57. 10.1016/S0925-4773(97)00125-1.View ArticlePubMedGoogle Scholar
- Feistel K, Blum M: Three types of cilia including a novel 9 + 4 axoneme on the notochordal plate of the rabbit embryo. Dev Dyn. 2006, 235: 3348-3358. 10.1002/dvdy.20986.View ArticlePubMedGoogle Scholar
- Klein SL: The first cleavage furrow demarcates the dorsal-ventral axis in Xenopus embryos. Dev Biol. 1987, 120: 299-304. 10.1016/0012-1606(87)90127-8.View ArticlePubMedGoogle Scholar
- Abràmoff MD, Magalhães PJ, Ram SJ: Image processing with imageJ. Biophotonics Int. 2004, 11: 36-42.Google Scholar
- Schindelin J, Arganda-Carreras I, Frise E, Kaynig V, Longair M, Pietzsch T, Preibisch S, Rueden C, Saalfeld S, Schmid B, Tinevez JY, White DJ, Hartenstein V, Eliceiri K, Tomancak P, Cardona A: Fiji: an open-source platform for biological-image analysis. Nat Methods. 2012, 9: 676-682. 10.1038/nmeth.2019.View ArticlePubMedGoogle Scholar
- Sbalzarini IF, Koumoutsakos P: Feature point tracking and trajectory analysis for video imaging in cell biology. J Struct Biol. 2005, 151: 182-195. 10.1016/j.jsb.2005.06.002.View ArticlePubMedGoogle Scholar
- Pohl BS, Knöchel W: Isolation and developmental expression of Xenopus FoxJ1 and FoxK1. Dev Genes Evol. 2004, 214: 200-205. 10.1007/s00427-004-0391-7.View ArticlePubMedGoogle Scholar
- Gaete M, Muñoz R, Sánchez N, Tampe R, Moreno M, Contreras EG, Lee-Liu D, Larraín J: Spinal cord regeneration in Xenopus tadpoles proceeds through activation of Sox2-positive cells. Neural Dev. 2012, 7: 13-10.1186/1749-8104-7-13.View ArticlePubMedPubMed CentralGoogle Scholar
- Domínguez L, González A, Moreno N: Sonic hedgehog expression during Xenopus laevis forebrain development. Brain Res. 2010, 1347: 19-32.View ArticlePubMedGoogle Scholar
- Mattes B, Weber S, Peres J, Chen Q, Davidson G, Houart C, Scholpp S: Wnt3 and Wnt3a are required for induction of the mid-diencephalic organizer in the caudal forebrain. Neural Dev. 2012, 7: 12-10.1186/1749-8104-7-12.View ArticlePubMedPubMed CentralGoogle Scholar
- Wullimann MF, Rink E, Vernier P, Schlosser G: Secondary neurogenesis in the brain of the African clawed frog, Xenopus laevis, as revealed by PCNA, Delta-1, Neurogenin-related-1, and NeuroD expression. J Comp Neurol. 2005, 489: 387-402. 10.1002/cne.20634.View ArticlePubMedGoogle Scholar
- Nieuwkoop PD: Normal table of Xenopus laevis (Daudin). 1967, New York, NY: Garland PublishingGoogle Scholar
- Vio K, Rodríguez S, Yulis CR, Oliver C, Rodríguez EM: The subcommissural organ of the rat secretes Reissner’s fiber glycoproteins and CSF-soluble proteins reaching the internal and external CSF compartments. Cerebrospinal Fluid Res. 2008, 5: 3-10.1186/1743-8454-5-3.View ArticlePubMedPubMed CentralGoogle Scholar
- Stubbs JL, Vladar EK, Axelrod JD, Kintner C: Multicilin promotes centriole assembly and ciliogenesis during multiciliate cell differentiation. Nat Cell Biol. 2012, 14: 140-147. 10.1038/ncb2406.View ArticlePubMedPubMed CentralGoogle Scholar
- Moody SA: Fates of the blastomeres of the 16-cell stage Xenopus embryo. Dev Biol. 1987, 119: 560-578. 10.1016/0012-1606(87)90059-5.View ArticlePubMedGoogle Scholar
- Moody SA: Fates of the blastomeres of the 32-cell-stage Xenopus embryo. Dev Biol. 1987, 122: 300-319. 10.1016/0012-1606(87)90296-X.View ArticlePubMedGoogle Scholar
- Bauer DV, Huang S, Moody SA: The cleavage stage origin of Spemann’s organizer: analysis of the movements of blastomere clones before and during gastrulation in Xenopus. Development. 1994, 120: 1179-1189.PubMedGoogle Scholar
- Mogi K, Adachi T, Izumi S, Toyoizumi R: Visualisation of cerebrospinal fluid flow patterns in albino Xenopus larvae in vivo. Fluids Barriers CNS. 2012, 9: 9-10.1186/2045-8118-9-9.View ArticlePubMedPubMed CentralGoogle Scholar
- Götz M, Huttner WB: The cell biology of neurogenesis. Nat Rev Mol Cell Biol. 2005, 6: 777-788. 10.1038/nrm1739.View ArticlePubMedGoogle Scholar
- Merkle F, Tramontin A, Garcia-Verdugo J, Alvarez-Buylla A: Radial glia give rise to adult neural stem cells in the subventricular zone. Proc Natl Acad Sci U S A. 2004, 101: 17528-17532. 10.1073/pnas.0407893101.View ArticlePubMedPubMed CentralGoogle Scholar
- Lim L, Zhou H, Costa RH: The winged helix transcription factor HFH-4 is expressed during choroid plexus epithelial development in the mouse embryo. Proc Natl Acad Sci U S A. 1997, 94: 3094-3099. 10.1073/pnas.94.7.3094.View ArticlePubMedPubMed CentralGoogle Scholar
- Banizs B, Pike MM, Millican CL, Ferguson WB, Komlosi P, Sheetz J, Bell PD, Schwiebert EM, Yoder BK: Dysfunctional cilia lead to altered ependyma and choroid plexus function, and result in the formation of hydrocephalus. Development. 2005, 132: 5329-5339. 10.1242/dev.02153.View ArticlePubMedGoogle Scholar
- Chung MI, Peyrot SM, LeBoeuf S, Park TJ, McGary KL, Marcotte EM, Wallingford JB: RFX2 is broadly required for ciliogenesis during vertebrate development. Dev Biol. 2012, 363: 155-165. 10.1016/j.ydbio.2011.12.029.View ArticlePubMedPubMed CentralGoogle Scholar
- Miskevich F: Imaging fluid flow and cilia beating pattern in Xenopus brain ventricles. J Neurosci Methods. 2010, 189: 1-4. 10.1016/j.jneumeth.2010.02.015.View ArticlePubMedGoogle Scholar
- Nelson DJ, Wright EM: The distribution, activity, and function of the cilia in the frog brain. J Physiol Lond. 1974, 243: 63-78.View ArticlePubMedPubMed CentralGoogle Scholar
- Gona AG, Hauser KF: Ultrastructural studies on the ventricular surface of the frog cerebellum. Cell Tissue Res. 1982, 225: 443-448.View ArticlePubMedGoogle Scholar
- Clary-Meinesz C, Mouroux J, Cosson J, Huitorel P, Blaive B: Influence of external pH on ciliary beat frequency in human bronchi and bronchioles. Eur Respir J. 1998, 11: 330-333. 10.1183/09031936.98.11020330.View ArticlePubMedGoogle Scholar
- Davy BE, Robinson ML: Congenital hydrocephalus in hy3 mice is caused by a frameshift mutation in Hydin, a large novel gene. Hum Mol Genet. 2003, 12: 1163-1170. 10.1093/hmg/ddg122.View ArticlePubMedGoogle Scholar
- Olbrich H, Schmidts M, Werner C, Onoufriadis A, Loges NT, Raidt J, Banki NF, Shoemark A, Burgoyne T, Turki AS, Hurles ME, Köhler G, Schroeder J, Nürnberg G, Nürnberg P, Chung EMK, Reinhardt R, Marthin JK, Nielsen KG, Mitchison HM, Omran H, UK10K Consortium: Recessive HYDIN mutations cause primary ciliary dyskinesia without randomization of left-right body asymmetry. Am J Hum Genet. 2012, 91: 672-684. 10.1016/j.ajhg.2012.08.016.View ArticlePubMedPubMed CentralGoogle Scholar
- Vio K, Rodríguez S, Navarrete EH, Pérez-Fígares JM, Jimenez AJ, Rodríguez EM: Hydrocephalus induced by immunological blockage of the subcommissural organ-Reissner’s fiber (RF) complex by maternal transfer of anti-RF antibodies. Exp Brain Res. 2000, 135: 41-52. 10.1007/s002210000474.View ArticlePubMedGoogle Scholar
- Ortloff AR, Vio K, Guerra M, Jaramillo K, Kaehne T, Jones H, McAllister JP, Rodríguez E: Role of the subcommissural organ in the pathogenesis of congenital hydrocephalus in the HTx rat. Cell Tissue Res. 2013, 352: 707-725. 10.1007/s00441-013-1615-9.View ArticlePubMedGoogle Scholar
- Lichtenfeld J, Viehweg J, Schutzenmeister J, Naumann WW: Reissner’s substance expressed as a transient pattern in vertebrate floor plate. Anat Embryol. 1999, 200: 161-174. 10.1007/s004290050270.View ArticlePubMedGoogle Scholar
- Amoyel M, Cheng YC, Jiang YJ, Wilkinson DG: Wnt1 regulates neurogenesis and mediates lateral inhibition of boundary cell specification in the zebrafish hindbrain. Development. 2005, 132: 775-785. 10.1242/dev.01616.View ArticlePubMedGoogle Scholar
- Cheng YC, Amoyel M, Qiu X, Jiang YJ, Xu Q, Wilkinson DG: Notch activation regulates the segregation and differentiation of rhombomere boundary cells in the zebrafish hindbrain. Dev Cell. 2004, 6: 539-550. 10.1016/S1534-5807(04)00097-8.View ArticlePubMedGoogle Scholar
- Riley BB, Chiang MY, Storch EM, Heck R, Buckles GR, Lekven AC: Rhombomere boundaries are Wnt signaling centers that regulate metameric patterning in the zebrafish hindbrain. Dev Dyn. 2004, 231: 278-291. 10.1002/dvdy.20133.View ArticlePubMedGoogle Scholar
- Pérez-Fígares JM, Jimenez AJ, Rodríguez EM: Subcommissural organ, cerebrospinal fluid circulation, and hydrocephalus. Microsc Res Tech. 2001, 52: 591-607. 10.1002/1097-0029(20010301)52:5<591::AID-JEMT1043>3.0.CO;2-7.View ArticlePubMedGoogle Scholar
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