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2905 Journal of Cell Science 110, 2905-2913 (1997) Printed in Great Britain © The Company of Biologists Limited 1997 JCS3646 Contact guidance of CNS neurites on grooved quartz: influence of groove dimensions, neuronal age and cell type Ann M. Rajnicek1,*, Stephen Britland2,3 and Colin D. McCaig1 1Department of Biomedical Sciences, Institute of Medical Sciences, University of Aberdeen, Aberdeen AB25 2ZD, 2Department of Electronics and Electrical Engineering, University of Glasgow, Glasgow, G12 8QQ, Scotland, UK 3Postgraduate Studies in Pharmacology, School of Pharmacy, University of Bradford, Bradford BD7 1DP, UK Scotland, UK *Author for correspondence (e-mail: [email protected]) SUMMARY We used an in vitro system that eliminates competing guidance cues found in embryos to determine whether substratum topography alone provides important neurite guidance information. Dissociated embryonic Xenopus spinal cord neurons and rat hippocampal neurons were grown on quartz etched with a series of parallel grooves. Xenopus neurites grew parallel to grooves as shallow as 14 nm and as narrow as 1 µm. Hippocampal neurites grew parallel to deep, wide grooves but perpendicular to shallow, narrow ones. Grooved substrata determined the sites at which neurites emerged from somas: Xenopus neurites sprouted from regions parallel to grooves but presumptive axons on rat hippocampal neurons emerged perpendicular to grooves and presumptive dendrites emerged parallel to them. Neurites grew faster in the favored direction of ori- entation and turned through large angles to align on grooves. The frequency of perpendicular alignment of hippocampal neurites depended on the age of the embryos from which neurons were isolated, suggesting that contact guidance is regulated in development. Collectively, the data indicate that substratum topography is a potent morphogenetic factor for developing CNS neurons and suggest that in addition to a role in pathfinding the geometry of the embryo assists in establishing neuronal polarity. In the companion paper (A. M. Rajnicek and C. D. McCaig (1997) J. Cell Sci. 110, 2915-2924) we explore the cellular mechanism for contact guidance of growth cones. INTRODUCTION topography, further suggesting that purely physical cues can direct neurite growth within embryos. In an effort to understand embryonic contact guidance events in vitro many cell types, including fibroblasts (Elsdale and Bard, 1972) and neurons (e.g. Ebendal, 1976) have been cultured on parallel arrays of aligned collagen fibrils or on parallel grooves manufactured in artificial substrata (Hirono et al., 1988; Clark et al., 1990; Oakley and Brunette, 1993). In most cases cells exhibit conventional contact guidance, aligning parallel to the groove/ridge axis, but even apparently simple contact guidance cues provide complex directional information to cells. For example, fibroblasts migrate unidirectionally on aligned collagen matrices (Boocock, 1989) and, depending on species and neuronal type, mammalian CNS neurites grow either parallel or perpendicular to aligned neurite bundles (Nagata and Nakatsuji, 1991) or artificial microstructures (Nagata et al., 1993). Contact guidance of cells by physical contours of the substratum was recognized in the earliest days of tissue culture (Harrison, 1914) yet surprisingly little is known about the cellular events of contact sensing and their transduction into directional growth, especially in neuronal growth cones. The aim of the present study was to describe the directional effects of substratum contours on the morphology of developing CNS neurons as a first step towards elucidating the mechanism for Contact guidance, the phenomenon by which the physical shape of the substratum induces alignment or directional growth of cells is involved in normal embryonic pattern formation (e.g. Newgreen, 1989). Nervous system development is influenced strongly by geometric patterns present within embryos during developmentally significant periods. For example, radial glia that span the walls of the developing brain are organized into regular arrays that foreshadow the route of migrating embryonic neurons (Hatten, 1990). In addition to a role in directional migration of cell bodies aligned cells also appear to guide process outgrowth. In the mammalian forebrain a ‘sling’ of subventricular cells forms a scaffold that predicts the trajectory of the corpus callosum (Schneider and Silver, 1990). Aligned channels that are subsequently invaded by pioneer axons exist in mouse (Silver and Sidman, 1980) and chick (Krayanek and Goldberg, 1981) optic stalk and dorsal retina. Similarly, the earliest fiber tracts in the Xenopus spinal cord form by ingrowth of axons into preexisting longitudinally oriented spaces between neuroepithelial cells of the neural tube (Nordlander and Singer, 1982a,b). Electron microscope studies of Xenopus embryos (Roberts and Taylor, 1983) demonstrate that even on a small scale growth cone morphology is influenced by substratum Key words: Topographic guidance, Growth cone, Hippocampal neuron, Xenopus neuron, Neuronal development, Substratum 2906 A. M. Rajnicek, S. Britland and C. D. McCaig topography-induced growth cone guidance. In the companion paper we explore the cellular mechanisms for contact guidance of growth cones (Rajnicek and McCaig, 1997b). MATERIALS AND METHODS Substrate preparation Microgrooved substrates were prepared from fused quartz using a direct writing electron beam lithographic process to etch a series of repeating, parallel grooves and ridges that were evenly spaced and had nearly right angle edges (Fig. 1A). The technique offers submicron precision in controlling grating periodicity beyond that attainable by conventional photolithographic microfabrication (Clark et al., 1990; Britland et al., 1996a). Eight experimental culture substrata, each comprising three 5 mm × 5 mm blocks of gratings with identical groove depths but different groove widths (1, 2 and 4 µm, respectively), were fabricated on one electron beam mask plate (Hoya, Japan). Each 6.5 cm square plate was composed of a 2 mm thick fused quartz base, a 100 nm chrome layer and 500 nm of EBR9 electron beam resist. The grating pattern was designed in WAM (an in-house microelectronic design package) and then translated into the BWL beam writing language format used by a Leica EBG5 Beamwriting machine which was operated with a 200 nm spot size at 50 kV. Beam current was automatically determined by spot size and resolution. Exposed resist was then developed using neat methyl iso-butyl ketone at room temperature and the underlying chrome removed by wet etching to reveal the quartz. The quartz base was then dry etched (RIE80, Plasma Technology, UK) using CHF3 plasma at 29 sccm (standard cubic centimeters per minute) flow rate and 15 mTorr and 100 W (rf) at 13.6 Mhz to give an etch rate of approximately 50 nm/minute. After removal of the remaining resist/chrome using acetone/chrome etch the substrates were blanket etched in CHF3 for 30 seconds using the parameters outlined above. Finally the mask plate was cut into 8 individual microscope slides using a diamond saw and the etch depth measured using Dektak and Talystep surface profilers. Two of the substrates were used for SEM and the remainder were used repeatedly for experimental purposes. Xenopus neurons were plated directly onto slides previously soaked overnight in concentrated nitric acid followed by several rinses with distilled water. Since these neurons prefer a minimal volume of growth medium, spacers made from narrow (~1 mm wide) strips of no. 1 thickness coverglass were secured to the long edges of the slides with MS4, a non-curing silicone compound (Dow Corning). Cells were plated into a small pool of culture medium in the central trough. After allowing ~30 minutes for the cells to adhere to the slide a coverslip that covered the entire quartz slide was secured on top to minimize evaporation. Slides were maintained at room temperature in a humidified atmosphere during the subsequent 6 to 9 hour growth period. For hippocampal neuron experiments the acid-cleaned slides were sterilized by UV irradiation and were then coated for 1 hour with 1 mg/ml poly-L-lysine (30-70 kDa; dissolved in sodium borate buffer, pH 8.5, immediately before use). Slides were then rinsed with sterile water and immersed grooved side up in a 60 mm Petri dish containing enough medium to completely submerge the slide (~4 ml). Cells were plated onto the slide without an overlying coverslip. For one experiment hippocampal neurons were plated onto polylysine-treated polystyrene replicas of etched surfaces (see photo in Fig. 5) completely submerged in culture medium. This surface comprised a series of adjoining 4 sided wells separated by narrow (~2 µm) walls with defined heights ranging from 0.118 µm to 3.16 µm. Neurites that stepped up, crossed over, then stepped down into the adjacent well were considered to have ‘crossed the step’. Cell culture Dissociated neurons from the neural tube of Xenopus laevis were cultured using a slight modification of a previously described culture method (Hinkle et al., 1981; McCaig et al., 1994). Neural tubes were dissected from several stage 20 Xenopus neurulae and pooled in calcium-magnesium-free Steinberg’s solution, pH 7.9, to disaggregate. The resulting cell suspension was triturated gently and then plated into a pool of culture medium in the central region of the slides described above. Culture medium was Steinberg’s solution (58 mM NaCl, 0.67 mM KCl, 0.44 mM Ca(NO3)2, 1.3 mM MgSO4 and 4.6 mM Tris-HCl, pH 7.9) supplemented with 20% Leibowitz’s L-15, 1% fetal bovine serum, 100 i.u./ml penicillin, 100 µg/ml streptomycin (all from ICN Biochemicals Ltd, Irvine, Scotland). Data were collected after 6 to 9 hours in culture at room temperature. Dissociated neurons from the E16 (and E19 for studies of age dependence) rat hippocampus were cultured in Earle’s minimal essential medium (MEM, Gibco) as described previously (Davenport and McCaig, 1993). After 3 hours the MEM containing 10% heat inactivated calf serum was replaced with MEM containing 10% Nu Serum V (Collaborative Research, Lexington, MA, USA). Data were collected from live cells after 24 hours in culture at 36°C, 5% CO2. Hippocampal cells were used fresh or were thawed from stocks frozen at −70°C in 8% DMSO (dimethylsulfoxide) by the method of Mattson and Kater (1988). Data from fresh and frozen cells were combined because there were no differences in their morphologies or directional responses. Data collection and analysis Measurements were made from live video images of cells using Leica Quantimet 500MC image collection and analysis software. For Xenopus neurons data were collected from each neurite but in the case of hippocampal neurons data were only collected from the longest neurite on each cell, which is the presumptive axon (Dotti et al., 1988). The angle of neurite orientation relative to the groove direction (θ) Fig. 1. (A) Scanning electron micrograph of a quartz microscope slide with grooves 520 nm deep and 2 µm wide. Note that the grooves have approximately right angled sides, sharp corners and are evenly spaced. The lower photo is a magnified view of the boxed region. (B) Angle measurement protocol for orientation assay. Angles were measured using computerized image collection and analysis software that allowed lines to be superimposed onto video images of cells. Images were always viewed with the groove/ridge axis horizontal. The direction of neurite growth was determined by a line connecting the neurite initiation site on the soma with the center of the growth cone. All angles measured were between 0° and 90°. Overall orientation for a population of neurites was determined by categorizing the angle of growth as ‘parallel’ to the grooves if θ was between 0° and 30° and ‘perpendicular’ if θ was between 60° and 90°. The mean percentage of neurites in each category was determined by pooling data for several sets of 50 cells grown under identical conditions. CNS neurite orientation on grooves 2907 was on grooves 1,100 nm deep and 4 µm wide. Orientation was not biased on flat quartz for either cell type. Most non-neuronal cells in hippocampal cultures aligned parallel to grooves of all dimensions. Grooved quartz slides were treated with polylysine before plating hippocampal neurons but not Xenopus neurons so we tested the notion that differences in orientation between the neuronal types was an artifact of polylysine treatment. Two lines of evidence argue that the differences are not related to polylysine treatment: (1) Xenopus neurites oriented parallel to grooves even when the slides were treated with polylysine (data not shown). The equivalent experiment, in which hippocampal neurons are grown on untreated quartz is impossible because polylysine treatment is required for hippocampal neuron differentiation. (2) Rat hippocampal neurites aligned either parallel or perpendicular to grooves depending on groove dimensions even though the substrates were always treated with polylysine. Parallel growth of neurites is not merely due to physical constraint within the grooves because individual growth cones often span several groove and ridge repeats (Figs 3D, 4A) and are therefore not confined by groove walls. Similarly, hippocampal neurites are able to cross single steps as high as 3.16 µm (Fig. 5) and would therefore be able to step out of grooves even deeper than those used in this study. Extrapolation of the data in Fig. 5 indicates that grooves would have to be 4.7 µm high to completely restrain hippocampal neurites. These data suggest that neurites make an active choice to grow either parallel or perpendicular to grooves. This idea is also supported by the observation that hippocampal neurites sometimes grew parallel to grooves before turning to grow across them (Fig. 4B). was determined as shown in Fig. 1B. Control (flat) data were collected from cells on the ungrooved regions of each etched slide. Angles were considered to be ‘parallel’ to the groove direction if θ was between 0° and 30° and angles were ‘perpendicular’ if θ was between 60° and 90°. The remainder of the neurites were classified as ‘intermediate’ and for the sake of clarity are not included in this report. The expected frequency in each category for a population of randomly oriented neurites is 33%. This was confirmed by measurements of the neurites grown on flat quartz surfaces. The percentage of neurites in each category was therefore compared to the control percentage for flat substrata using a d-test (Bailey, 1981) or one way ANOVA followed by a Dunnet multiple comparison test. RESULTS The direction of CNS neurite orientation depends on cell type and groove dimensions Dissociated neurons from embryonic Xenopus spinal cord and embryonic rat hippocampus revealed strikingly different growth patterns on grooved surfaces (Figs 2, 3). Xenopus spinal neurites exhibited classical contact guidance by growing parallel to grooves with depths ranging from 14 nm to 1,100 nm and widths of 1, 2 or 4 µm (Fig. 2A). By contrast, hippocampal neurites showed a more complex response. In general they grew perpendicular to shallow, narrow grooves and parallel to deep, wide ones (Fig. 2B). At certain groove depths (130 nm, 520 nm, and 1,100 nm) hippocampal neurites changed their direction of growth from perpendicular on grooves 1 µm and 2 µm wide to parallel on grooves 4 µm wide even though the groove depth was unchanged. The greatest perpendicular response for hippocampal neurites was on grooves 130 nm deep and 1 µm wide and the greatest parallel response A Xenopus spinal neurites parallel 100 % neurites 80 1 µm * B perpendicular ** parallel ** ** ** 100 * * 20 40 ** ** ** ** ** ** * ** ** * ** 0 14 36 2 µm ** 100 % neurites ** 20 ** ** 0 ** 130 140 520 ** 1100 ** 14 ** ** 100 36 60 40 ** ** ** ** 520 ** ** 1100 ** ** * 40 ** 140 2 µm 60 ** 130 80 0 * 20 0 14 36 * 4 µm ** 100 80 % neurites 1 µm 60 40 20 perpendicular 80 60 80 rat hippocampal neurites 130 140 ** ** 520 ** 1100 ** 14 100 4 µm 80 60 36 130 140 520 ** ** ** 1100 60 40 40 ** 20 ** ** ** ** 0 * 20 * 0 14 36 130 140 groove depth (nm) 520 1100 14 36 130 140 groove depth (nm) 520 1100 Fig. 2. Orientation responses of (A) Xenopus spinal cord neurites and (B) rat hippocampal neurites on grooved substrata. The direction of neurite growth was measured as shown in Fig. 1B and is presented as the mean percentage of total neurites parallel (white bars) or perpendicular (black bars) to the groove direction ± sd. The groove width is indicated in the upper left of each graph. Data were pooled from at least two experiments on each substrate. The number of Xenopus neurites on grooves ranged from 93 (on 130 nm deep, 4 µm wide grooves) to 188 (on 140 nm deep, 1 µm wide grooves). The number of hippocampal neurites ranged from 100 (on 14 nm and 520 nm grooves) to 400 (on 130 nm deep, 1 µm wide grooves). Asterisks represent values significantly different from the measured control frequencies of 34±3% parallel and 33±3% perpendicular for Xenopus (n=300) and 34±6% parallel and 34±5% perpendicular for hippocampal neurites (n=750) on flat quartz (*P<0.05, **P<0.01 by one way ANOVA). These control frequencies were not different from 33% (d-test, Bailey, 1981), which is the expected freqency of parallel or perpendicular neurites in a randomly oriented population. 2908 A. M. Rajnicek, S. Britland and C. D. McCaig Fig. 3. Phase contrast micrographs of E16 rat hippocampal neurons (A and B) and Xenopus spinal cord neurons (C and D). Rat and Xenopus neurons had been growing for 24 and 4 hours, respectively. Cells are growing on flat quartz (A and C) or on grooves 1 µm wide and 130 nm deep (B) or 320 nm deep (D). In phase contrast micrographs of grooved surfaces the ridges appear as phase dark stripes and the grooves appear as phase bright stripes. Bars: (A,B) 50 µm; (C,D) 100 µm. Grooved substrata determine the sites at which neurites emerge from somas Neurons were grown on grooved substrates to test whether topographical features of the substratum determined aspects of neuronal morphology even more subtle than the direction of overall neurite extension. In particular we examined the direction of neurite initiation, direction of turning and the rate of neurite elongation. Grooved substrata determined the site on the soma that gave rise to neurites. Neurites were uniformly distributed on flat quartz or on grooves 14 nm deep but most Xenopus neurites emerged from regions of the somas parallel to grooves greater than 36 nm deep (Figs 6A, 7C). Hippocampal neurites showed a more varied response (Fig. 6B). One day after plating hippocampal neurons generally bear one long process that becomes the axon and several shorter, minor processes that subsequently become dendrites (Dotti et al., 1988). By these criteria most presumptive axons emerged from perpendicular regions and presumptive dendrites emerged from parallel regions of hippocampal somas on grooves. Presumptive dendrites maintained parallel growth as they extended (Fig. 3B). This implies that the physical contour of the environment influences the fine structural, and therefore functional, polarity of differentiating hippocampal neurons. Fig. 4. Neurites turn in relation to the groove direction. (A) Phase contrast micrograph of Xenopus neurites on grooves 14 nm deep and 1 µm wide. Cells were plated 8 hours previously. At least three neurites (arrows) turned through large angles to grow parallel to the grooves. In one case (double arrows) two neurites appear to have fasciculated yet they still turn to be parallel. Note that neurite initiation sites are not biased by the 14 nm grooves. Bar, 50 µm. (B) Differential interference micrograph of a hippocampal neuron whose cell body rests on flat quartz (left side of photo). As the neurite encounters the grooved region of the slide it turns abruptly (arrow) to become perpendicular to the 140 nm deep, 1 µm wide grooves. Bar, 50 µm. Neurites turn to grow in the preferred orientation Neurites of both cell types often adjust their trajectories by turning toward their preferred direction of orientation. For example, Xenopus neurites on substrates with grooves 14 nm deep and 1 µm wide are symetrically distributed around the soma (Figs 4A, 6A) yet they demonstrate parallel contact guidance on these grooves (Fig. 2A). This suggests that Xenopus neurites change direction as they grow in order to align parallel to grooves. Observations of single neurons support this notion (Figs 4A, 8). Although most presumptive axons on hippocampal neurons emerged from regions of cell bodies perpendicular to grooves (Fig. 6B) the degree of turning relative to the groove direction was assessed to determine whether they would turn to align perpendicular to grooves. These observations were made on grooves 130 nm deep and 1 µm across, which is the substrate that elicited maximum (85±6%) perpendicular orientation (Fig. 2B). Turning was defined as a deviation of 15° or more by the distal (growth cone) end of a neurite relative to the proximal end (nearest the soma) of the same neurite. On flat quartz neurites turned uniformly in all directions: 32% toward grooves, 33% away from grooves and 43% do not turn (n=200) but on grooved surfaces more than twice as many turned away from the direction of the grooves (46%) than turned toward CNS neurite orientation on grooves 2909 tively. The etched regions were surrounded by flat regions used for control measurements. Collecting data from a single slide excluded the potential effects of variation in substratum surface chemistry and day to day variation in growth. On grooves 1 or 2 µm wide neurites aligned mostly perpendicular to grooves (Fig. 2B) and were longer than those aligned parallel on the same substrate (Fig. 9). On grooves 4 µm wide, however, neurite orientation was random (Fig. 2B) and the length perpendicular was not different from that parallel or that on flat quartz (Fig. 9). The mean length of neurites parallel to grooves (regardless of width) were the same as those on flat quartz. Neurite length (hence, net growth rate) is therefore increased selectively in neurites growing perpendicular to grooves. Neurites grow faster in the preferred orientation on grooves In general neurites grew faster in their preferred orientation than in less favored directions or on flat quartz. Xenopus neurites growing parallel to 130 nm deep, 1 µm wide grooves (26±1.6 µm/hour, mean ± s.e.m., n=15) grew significantly faster (P<0.0001, 2-tailed Student’s t-test) than those oriented randomly on flat quartz (14±0.6 µm/hour, n=74). Since all neurites grew parallel to grooves in these time lapse experiments no comparison could be made with growth rates of neurites on grooved substrata extending in less preferred orientations. Hippocampal neurites showed a similar tendency to grow faster in the preferred orientation. For example, on the substratum that elicited maximum perpendicular orientation (130 nm deep, 1 µm wide grooves) hippocampal neurites perpendicular to grooves were longer than those parallel to grooves and those on flat quartz (Fig. 9). Neurites on flat quartz had uniform lengths regardless of orientation (Fig. 9). Since length measurements were made 24 hours after plating in each case this suggests that the net rate of neurite growth was increased for hippocampal neurites growing across grooves. This conclusion was confirmed by measuring hippocampal neurite lengths on a slide containing three etched regions with grooves 140 nm deep but widths of 1, 2 or 4 µm in each region, respec- A 100 % initiation sites them (16%) and 38% did not turn (n=100). The mean angle turned away from grooves (35±3°) was greater (P=0.0074, 2tailed t-test) than that turned toward grooves (25±2°). Hippocampal neurites were therefore able to correct their course away from the groove/ridge direction to grow across, rather than along grooves. In some cases neurites on flat regions of the slides happened to grow onto the grooved region, changing course abruptly to grow perpendicular to grooves (Fig. 4B). This observation further supports the notion that perpendicular orientation on these surfaces is an active choice. Embryonic age and species affect perpendicular alignment of hippocampal neurons Cells dissociated from rat hippocampi of different embryonic ages were grown on 130 nm deep grooves to explore the temporal developmental significance of contact guidance. Perpendicular orientation on 1 or 2 µm wide grooves was greater for neurons isolated from E16 hippocampi than for those from E19 hippocampi (Fig. 10). E16 neurites aligned perpendicular at 1 and 2 µm widths but E19 neurites shifted from perpendicular orientation at 1 µm repeats to parallel orientation at 2 µm repeats (Fig. 10). Although hippocampal neurons isolated from E16 mice or rats show predominantly perpendicular orientation on 130 nm deep, 1 µm wide grooves those isolated from mice are less Xenopus neurons 80 *** *** *** parallel perpendicular 60 40 * 20 ** *** 0 flat 14 36 140 groove depth (nm) 320 *** 520 B B % initiation sites Fig. 5. Hippocampal growth cones crossed ridges as high as 3.16 µm. There is a direct correlation between ridge height and the frequency of neurites that cross over them (R2 = 0.9898). Extrapolation of the line indicates that ridges would have to be at least 4.7 µm high to prevent all neurites from crossing. Asterisks indicate values significantly different from 100%. *0.05≥P≥0.02; **P<0.001 (d-test; Bailey, 1981). The number of neurites measured ranged from 36 to 50 at each height. Inset shows a hippocampal neuron a substratum with ridges (phase dark lines) 0.27 µm high. Note that both growth cones have crossed the ridges. 60 hippocampal neurons *** * parallel perpendicular 40 ** 20 ** 0 presumptive axons presumptive dendrites flat presumptive axons presumptive dendrites grooved Fig. 6. Effect of substratum contour on the site at which neurites sprout on cell bodies. All grooves were 1 µm wide. The dashed lines indicate the expected control frequency for randomly oriented neurites on flat quartz. Asterisks indicate values that are significantly different than those on flat surfaces by a d test (Bailey, 1981) *0.05>P>0.02; **0.02>P>0.01; ***P<0.001. (A) For Xenopus neurons data were collected 2.5 hours after plating and n was 250 for flat and 50 for each grooved substrate. (B) For hippocampal neurons initiation sites were measured 24 hours after plating on 130 nm deep grooves. Data were pooled from 3 experiments. The longest neurite on each cell was the presumptive axon and the minor processes were the presumptive dendrites (Dotti et al., 1988). On flat quartz n=50 presumptive axons and 104 presumptive dendrites; on grooves n=135 presumptive axons and 333 presumptive dendrites. 2910 A. M. Rajnicek, S. Britland and C. D. McCaig Fig. 8. Xenopus neurons that landed fortuitously at the boundary between grooved regions (right) and flat regions (left) of the slides during plating. Grooves are 1 µm wide and 320 nm deep (A) or 520 nm deep (B). Note that for each cell neurites on grooves are straighter and longer than those on the flat region. Bar, 50 µm. Fig. 7. Time lapse photos of Xenopus neurons on grooves 140 nm deep and 1 µm wide. (A) The first photo (T = 0 hours) was taken 4 hours after plating. (B) 2 hours later. (C) 4 hours later. Arrows indicate branch points that resulted from growth cone bifurcation. Asterisks in (C) indicate newly differentiating cells. Note that neurites emerge parallel to the groove/ridge axis. Bar, 50 µm. likely to exhibit perpendicular alignment. After 24 hours in culture 81±2% of E16 rat neurites (Fig. 10) but only 50±6% (mean ± s.d., n=100) of E16 mouse neurites aligned perpendicular to grooves (P=0.003, 2 tailed Student’s t-test). This reduction could reflect species differences or differences in the relative rates of mouse and rat hippocampal development because hippocampal development in the mouse begins earlier (E10) than in the rat (E15) and the development of Ammon’s horn is more protracted in the mouse than the rat (Reznikov, 1991). The frequency of perpendicular alignment of E16 mouse neurites was therefore compared to E19 rat neurites, which may be more similar developmentally. There was no difference (Student’s t-test) between the frequency of perpendicular alignment for E16 mouse neurons (50±6%, n=100) compared to E19 rat neurons (61±7%, n=150). DISCUSSION The nature of various attractive, repulsive, permissive and inhibitory characteristics of neuronal pathways has received much attention in the context of growth cone guidance (reviewed by Keynes and Cook, 1995a,b; Tessier-Lavigne and Goodman, 1996). It is likely that interplay between multiple factors is required for axon guidance and correct target recog- nition. Guidance by substratum contours has been largely overlooked and is usually treated as incidental but evidence that spaces precede outgrowth of some CNS neurons during development and regeneration (e.g. Singer et al., 1979), that CNS neurites are guided by radial glial cells (e.g. Norris and Kalil, 1991) and that substratum topography affects growth cone shape (Harris et al., 1985; Nordlander et al., 1991) suggest collectively that guidance by topographical features warrants investigation in its own right. Topographical guidance may be important during hippocampus development because alveolar channels in the embryonic rat hippocampus are presumed to guide pyramidal axons (Altman and Bayer, 1990b) and non-pyramidal neurons in the hippocampus may provide contact guidance for later outgrowing septohippocampal fibers (Supèr and Soriano, 1994). Additionally, Cajal described hippocampal mossy fibers as being grooved into the irregularities of the surface of regio inferior neurons suggesting a relationship between topography and neurite paths (Blackstad and Kjaerheim, 1961). We used an in vitro system that eliminated simultaneous presentation of potentially competitive guidance cues to explore the contribution of the physical shape of the substratum in neuronal morphogenesis. Our data indicate that substratum contours provide important morphogenetic information to developing CNS neurons in an age-dependent way by influencing the site of neurite initiation on somas, the direction of neurite growth (determined by groove dimensions), the presumptive axonal or dendritic identity of neuronal processes and the rate of neurite elongation. The increase in net perpendicular growth rate on narrow grooves is selective because neurites that grow parallel to the same grooves are significantly shorter than perpendicular ones but no different than those on flat quartz. The net increase could be due to enhanced trophic support for neurites on grooves because of the increased CNS neurite orientation on grooves 2911 100 parallel perpendicular *** 100 ** 80 E16 *** *** 80 * % neurites length+sem (µm) 120 60 40 0 perpendicular *** 60 * ** 40 20 20 parallel E19 *** *** 0 flat 130×1 140×1 140×2 140×4 groove depth (nm)×width (µm) Fig. 9. Rat hippocampal neurites are longer when aligned perpendicular to grooves than when they are parallel or on flat substrates. All data were collected 24 h after plating and are expressed as mean neurite length ± s.d. Astersisks indicate significant differences in the length of neurites growing perpendicular compared to those growing parallel on the same substrate; *P=0.0261, **P=0.0012, ***P<0.0001 (2-tailed Student’s t-test). Number of neurites measured on each substrate (parallel and perpendicular, respectively): on flat quartz n=32 and 32, on 130 nm × 1µm grooves n=18 and 91, on 140 nm × 1 µm grooves n=16 and 68, on 140 nm × 1 µm grooves n=27 and 49, and on 140 nm × 4 µm grooves n=30 and 40. At a width of 1 µm there is no difference in the length of neurites perpendicular to grooves 130 nm deep compared to those perpendicular on 140 nm deep grooves. Neurite length on grooves 140 nm deep and 4 µm wide is not different from that on flat quartz. Neurites oriented parallel to grooves 130 nm deep and 1 µm wide were shorter (P=0.0327) than parallel neurites on flat quartz. membrane surface area exposed to nutrient-rich culture medium. This does not appear to be the case however because on grooved surfaces that induce random orientation neurite length is the same as that on flat quartz. This suggests that perpendicular neurite growth rate is stimulated only on grooved surfaces that stimulate perpendicular orientation. Alignment on grooved surfaces appears to be an active process Neurites changed their direction of growth to reflect their preferred orientation on grooves. Xenopus neurites monitored over time adjusted their trajectories, turning parallel to grooves. Whilst only 16% of hippocampal neurites turned parallel to grooves that induced perpendicular alignment, 46% turned away from grooves (and through larger angles), yielding perpendicular orientation. Control experiments ruled out the possibility that perpendicular orientation was related to polylysine treatment of the growth surface. Xenopus and hippocampal neurites grew parallel to grooves too small to restrain them physically, suggesting that parallel orientation is not merely due to neurites being trapped within grooves. This idea is supported by the observation that hippocampal neurites climbed over steps at least 3 times higher than those that induced parallel orientation. These observations suggest collectively that alignment on grooved substrata is an active rather than passive event. Contact guidance by neurons in situ Xenopus spinal neurons and rat hippocampal neurons were used in the present investigation because evidence from anatomical studies of Xenopus spinal cord and mammalian brain, including the hippocampus suggest that surface contours affect the pattern 130×1 130×2 130×1 130×2 groove depth (nm)×width (µm) Fig. 10. Age dependent differences in orientation on grooves. Hippocampal neurons were isolated from E16 (left side of figure) or E19 (right side of figure) rat embryos. Perpendicular contact guidance was enhanced for E16 neurites compared to E19 (P=0.0089 and P=0.0035 for E16 versus E19 neurons at 1 and 2 µm widths, respectively by a 2-tailed Student’s t-test). On 130 nm × 1 µm substrates the number of neurites was 150 at E16 and 150 at E19. On 130 nm × 2 µm the number of neurites was 50 at E16 and 100 at E19. Asterisks indicate differences between the percentage parallel or perpendicular compared to a control value of 34% for flat quartz (dashed line); *0.01<P<0.02, **0.0001<P<0.001, ***P<0.0001 by a 2-tailed Student’s t-test. of neurite growth. For example, in the Xenopus spinal cord sensory ganglion neurons grow along tracts of preexisting, longitudinally aligned Rohon-Beard neurons (Nordlander et al., 1991) and aligned spaces between neighboring neuroepithelial cells form channels which the earliest axonal outgrowths subsequently invade (Nordlander and Singer, 1982a,b). Published electron micrographs (e.g. Fig. 2 of Nordlander and Singer, 1982a) indicate that the channels range from approximately 0.6 µm to 3 µm across. Even the smallest spaces are therefore at least five times larger than the minimum groove depth that induced parallel orientation of Xenopus spinal cord neurites (our Fig. 2A). The first spaces to appear in the Xenopus spinal cord form adjacent to the differentiating Rohon-Beard neurons (Nordlander and Singer, 1982a). Cultures of dissociated neural tubes yield a heterogeneous population of sensory neurons (e.g. Rohon-Beard neurons), motor neurons and interneurons (Tabti and Poo, 1991). Since greater than 80% of Xenopus neurites grew parallel to grooves 130 nm deep and deeper in our experiments (Fig. 4A) it is probable that the majority of embryonic spinal cord neurons, including RohonBeard neurons, would align with parallel topographical features in situ. Indeed, growth cones of Xenopus sensory ganglion neurons appear to be directed by the geometry of their surroundings so that axons, their growth cones and filopodia align parallel to the dorsolateral fasciculus (Nordlander et al., 1991). The highly stereotyped crisscross pattern of neuronal processes within the mammalian hippocampus was noted during the early histological studies by Santiago Ramón y Cajal (1893) but the mechanism that generates such striking geometry has not been established clearly. The adult mammalian hippocampus is one of the most widely studied brain structures (Reznikov, 1991) largely because of its well defined neuronal circuitry, yet little effort has been made to determine how appropriate connections are established during development. Most in situ studies of embryonic hippocampal development have concentrated on neurogenesis (‘birth dates’ and migration patterns 2912 A. M. Rajnicek, S. Britland and C. D. McCaig of undifferentiated neurons) rather than on the process of axon outgrowth per se (e.g. Bayer, 1980; Altman and Bayer, 1990a). It would be instructive to identify factors that determine fiber outgrowth patterns in the hippocampus because they may also be relevant to other brain regions. This seems likely because neurites from a variety of mammalian CNS regions exhibit perpendicular contact guidance on parallel arrays of neurites (Hekmat et al., 1989; Nagata and Nakatsuji, 1991) and artificial microstructures in vitro (Nagata et al., 1993). Although Nagata et al. (1993) state that mouse E17-18 hippocampal neuroblasts showed ‘relatively higher frequency of parallel orientation’ on grooved quartz it is difficult to compare our results with theirs directly because no data were provided for hippocampal neurons. Our study extends that of Nagata et al. (1993) to indicate that grooved substrata determine the rate of neurite extension and the direction of presumptive axon or dendrite initiation as well as the direction of neurite growth. Relevance of contact guidance to development and regeneration Our data that neurons from hippocampi of different embryonic ages respond differently to identical topographical guidance cues support the notion that contact guidance acts during hippocampus development by suggesting that the ability to respond to topographical cues is regulated temporally. Our data do not indicate whether the temporal differences reflect changes in the types of neurons present in the cultures at different embryonic ages or changes in the responsiveness of individual neuronal types. Hippocampal development in the rat begins at E15 and development of Ammon’s horn is most rapid between E17-19 (Reznikov, 1991). It is likely therefore that E16 cultures contain a smaller proportion of pyramidal neurons, which may represent as much 80-85% (probably from fields CA1, or CA2-CA4) of the population in E19 cultures (Banker and Cowan, 1979). This variation in cellular composition may account for the age-related decrease in perpendicular orientation of E19 compared to E16 cultures. However, neurons of the same age, from the same cell suspension respond orthogonally to substrata differing only in groove width. This indicates that subtle variations in embryonic geometry have profound effects on neuronal morphology and suggests that topographic cues encode more complex guidance information than they are generally attributed with. Anatomically aligned spaces exist in the developing and in the regenerating spinal cord of newts and lizards (Singer et al., 1979) and growth cones often grow along other neurites during development and regeneration (Nordlander et al., 1991). Indeed, some procedures aimed at enhancing CNS regeneration have exploited this observation by using carbon filaments as substrates for contact guidance of regenerating nerve fibers (Khan et al., 1991). Our data indicate that the dimensions of substrata used for such treatments are crucial if they are to produce effective guidance of CNS neurites across lesion sites. Possible interactions with other guidance cues We do not propose that guidance of neurites by physical substratum cues alone explains axonal guidance to targets but it is likely that contact guidance acts in concert with other neuronal stimulatory and inhibitory growth cone guidance factors. For example, steady, DC electric fields associated with the amphibian neural tube (Hotary and Robinson, 1991; Shi and Borgens, 1994) and the mammalian primitive streak been implicated in neuronal morphogenesis (Winkel and Nuccitelli, 1989; Hotary and Robinson, 1992; Shi and Borgens 1994). Interestingly, Xenopus spinal neurites in weak, DC electric fields respond parallel to the electric field lines (see McCaig et al., 1994, for review) and rat hippocampal neurites respond perpendicular to them (Rajnicek et al., 1992), thus mimicing their respective contact guidance preferences in the present study. On shallow grooved substrata with an overlying orthogonal adhesive track chick dorsal root ganglion neurites aligned preferentially on the adhesive tracks but on deeper grooves they ignored the adhesive paths and aligned parallel to grooves (Britland et al., 1996b). Similar competition experiments have not been done using mammalian CNS neurons. Future experiments will therefore examine the heirarchy of CNS guidance cues by establishing competing gradients of electrical cues, substratum gradients of tropic molecules and gradients of soluble chemoattractants. In summary, CNS neurites are very sensitive to topographical contact guidance cues in the absence of simultaneous chemical or electrical gradients. Xenopus neurites grew parallel to grooves but hippocampal neurites regulated their direction of neurite growth depending on groove dimensions and developmental age. Grooved substrata influenced the site at which neurites emerged from cell bodies, the presumptive axonal or dendritic identity of neurites, the direction of neurite growth and the rate of neurite elongation. Taken together, these data suggest that perpendicular alignment has at least three contributing factors: (1) Presumptive axons emerge perpendicular to the groove/ridge axis. (2) Neurites turn more frequently and through larger angles to grow across, rather than along grooves. (3) Neurites grow more quickly across grooves than parallel to them or on flat substrata. The companion paper (Rajnicek and McCaig, 1997) addresses the question of how growth cones sense small surface contours and the signal transduction events that lead to directional growth. This work was supported by the Wellcome Trust (A.M.R. and C.D.McC.) and EPSRC (S.B.). Polystyrene replica substrates were a generous gift from Harvey Hoch at Cornell University (USA). We acknowledge the assistance of Chris Wilkinson, Department of Electronics and Electrical Engineering, Glasgow University and especially the technical assistance of Bill Monaghan at Glasgow University for advice and assistance with the fabrication of grooved substrata. REFERENCES Altman, J. and Bayer, S. A. (1990a). Mosaic organization of the hippocampal neuroepithelium and the multiple germinal sources of dentate granule cells. J. Comp. Neurol. 301, 325-342. Altman, J. and Bayer, S. A. (1990b). Prolonged sojourn of developing pyramidal cells in the intermediate zone of the hippocampus and their settling in the stratum pyramidale. J. Comp. Neurol. 301, 343-346. Bailey, N. T. J. (1981). In Statistical Methods in Biology, 2nd edn, pp. 38-39. Hodder and Stoughton, London. Banker, G. A. and Cowan, M. W. (1979). Further observations on hippocampal neurons in dispersed cell culture. J. Comp. Neurol. 187, 469-494. Bayer, S. A. (1980). Development of the hippocampal region in the rat: I. Neurogenesis examined with 3H-thymidine autoradiography. J. Comp. Neurol. 190, 87-114. Blackstad, T. W. and Kjaerheim, Å. (1961). Special axo-dendritic synapses in the hippocampal cortex: electron and light microscopic studies on the layer of mossy fibers. J. Comp. Neurol. 117, 133-159. Boocock, C. A. (1989). Unidirectional displacement of cells in fibrillar matrices. Development 107, 881-890. Britland, S., Morgan, H., Wojiak-Stodart, B., Riehle, M., Curtis, A. and CNS neurite orientation on grooves 2913 Wilkinson, C. (1996a). Synergistic and hierarchical adhesive and topographic guidance of BHK cells. Exp. Cell Res. 228, 313-325. Britland, S., Perridge, C., Denyer, M., Morgan, H., Curtis, A. and Wilkinson, C. (1996b). Morphogenetic guidance cues can interact synergistically and hierarchically in steering nerve cell growth. Exp. Biol. Online 1:2 (http://www. science. springer. de). Clark, P., Connolly, P., Curtis, A. S. G., Dow, J. A. T. and Wilkinson, C. D. (1990). Topographical control of cell behaviour: II. multiple grooved substrata. Development 108, 635-644. Davenport, R. W. and McCaig. C. D. (1993). Hippocampal growth cone responses to focally applied electric fields. J. Neurobiol. 24, 89-100. Dotti, C. G., Sullivan, C. A. and Banker, G. A. (1988). The establishment of polarity by hippocampal neurons in culture. J. Neurosci. 8, 1454-1468. Ebendal, T. (1976). The relative roles of contact inhibition and contact guidance in orientation of axons extending on aligned collagen fibrils in vitro. Exp. Cell Res. 98, 159-169. Elsdale, T. and Bard, J. (1972). Collagen substrata for studies on cell behavior. J. Cell Biol. 54, 626-637. Harris, W. A., Holt, C. E., Smith, T. A. and Gallenson, M. (1985). Growth cones of developing retinal cells in vivo, on culture surfaces and in collagen matrices. J. Neurosci. Res. 13, 101-122. Harrison, R. G. (1914). The reaction of embryonic cells to solid structures. J. Exp. Zool. 17, 521-544. Hatten, M. E. (1990). Riding the glial monorail: a common mechanism for glial-guided neuronal migration in different regions of the developing mammalian brain. Trends Neurosci. 13, 179-181. Hekmat, A., Künemund, V., Fischer, G., and Schachner, M. (1989). Small inhibitory cerebellar interneurons grow in a perpendicular orientation to granule cell neurites in culture. Neuron 2, 1113-1122. Hinkle, L., McCaig, C. D. and Robinson, K. R. (1981). The direction of growth of differentiating neurones and myoblasts from frog embryos in an applied electric field. J. Physiol. 314, 121-135. Hirono, T., Torimitsu, K., Kawana, A. and Fukuda, J. (1988). Recognition of artificial microstructures by sensory nerve fibers in culture. Brain Res. 446, 189-194. Hotary, K. B. and Robinson, K. R. (1991). The neural tube of the Xenopus embryo maintains a potential difference across itself. Dev. Brain Res. 59, 65-73. Hotary, K. B. and Robinson, K. R. (1992). Evidence of a role for endogenous electrical fields in chick embryo development. Development 114, 985-996. Khan, T., Dauzvardis, M. and Sayers, S. (1991). Carbon filament implants promote axonal growh across the transected rat spinal cord. Brain Res. 541, 139-145. Keynes, R. J. and Cook, G. M. W. (1995a). Repulsive and inhibitory signals. Curr. Opin. Neurobiol. 5, 75-82. Keynes, R. J. and Cook, G. M. W. (1995b). Axon guidance molecules. Cell 83, 151-169. Krayanek, S. and Goldberg, S. (1981). Oriented extracellular channels and axonal guidance in the embryonic chick retina. Dev. Biol. 84, 41-50. Mattson, M. P. and Kater, S. B. (1988). Isolated hippocampal neurons in cryopreserved long-term cultures: development of neuroarchitechture and sensitivity to NMDA. Int. J. Dev. Neurosci. 6, 439-452. McCaig, C. D., Allan, D. W., Erskine, L. E., Rajnicek, A. M. and Stewart, R. (1994). Growing nerves in an electric field. Neuroprotocols 4, 143-141. Nagata, I. and Nakatsuji, N. (1991). Rodent CNS neuroblasts exhibit both perpendicular and parallel contact guidance on the aligned parallel neurite bundle. Development 112, 581-590. Nagata, I., Kawana, A. and Nakatsuji, N. (1993). Perpendicular contact guidance of CNS neuroblasts on artificial microstructures. Development 117, 401-408. Newgreen, D. F. (1989). Physical influences on neural crest migration in avian embryos: contact guidance and spatial restriction. Dev. Biol. 131, 136-148. Nordlander, R. H. and Singer, M. (1982a). Spaces precede axons in Xenopus embryonic spinal cord. Exp. Neurol. 75, 221-228. Nordlander, R. H. and Singer, M. (1982b). Morphology and position of growth cones in the developing Xenopus spinal cord. Dev. Brain Res. 4, 181-193. Nordlander, R. H., Gazzerro, J. W. and Cook, H. (1991). Growth cones and axon trajectories of a sensory path in the amphibian spinal cord. J. Comp. Neurol. 307, 539-548. Norris, C. R. and Kalil, K. (1991). Guidance of callosal axons by radial glia in the developing cerebral cortex. J. Neurosci. 11, 3481-3492. Oakley, C. and Brunette, D. M. (1993). The sequence of alignment of microtubules, focal contacts and actin filaments in fibroblasts spreading on smooth and titanium substrata. J. Cell Sci. 106, 343-354. Rajnicek, A. M., Gow, N. A. R. and McCaig, C. D. (1992). Electric fieldinduced orientation of rat hippocampal neurones in vitro. Exp. Physiol. 77, 229-232. Rajnicek, A. M. and McCaig, C. D. (1997). Guidance of CNS growth cones by substratum grooves and ridges: effects of inhibitors of the cytoskeleton, calcium channels and signal transduction pathways. J. Cell Sci. 110, 2915-2924. Ramón y Cajal, S. (1893). The Structure of Ammon’s horn (English translation by L. M. Kraft, 1968). 78 pp. Charles C. Thomas, Springfield. Reznikov, K. (1991). Hippocampal formation in the mouse and rat – structural and organization and development: a review. In Cell Proliferation and Cytogenesis in the Mouse Hippocampus (ed. F. Beck, W. Hild, W. Kriz, J. E. Pauly, Y. Sano and T. H. Schiebler), pp. 1-81. Springer-Verlag, Roberts, A. and Taylor, J. S. H. (1983). A study of the growth cones of developing embryonic sensory neurites. J. Embryol. Exp. Morphol. 75, 3147. Schneider, B. F. and Silver, J. (1990). Failure of the subcallosal sling to develop after embryonic X-irradiation is correlated with absence of the cavum septi. J. Comp. Neurol. 299, 462-469. Shi, R. and Borgens, R. B. (1994). Embryonic neuroepithelial sodium transport, the resulting physiological potential, and cranial development. Dev. Biol. 165, 105-116. Silver, J. and Sidman, R. L. (1980). A mechanism for the guidance and topographic patterning of retinal ganglion cell axons. J. Comp. Neurol. 189, 101-111. Singer, M., Nordlander, R. H. and Egar, M. (1979). Axonal guidance during embryogenesis and regeneration in the spinal cord of the newt: the blueprint hypothesis of neuronal pathway patterning. J. Comp. Neurol. 185, 1-22. Supèr, H. and Soriano, E. (1994). The organization of the embryonic and early postnatal murine hippocampus. II. Development of entorhinal, commissural and septal connections studied with the lipophilic tracer DiI. J. Comp. Neurol. 344, 101-120. Tabti, N. and Poo, M.-m. (1991). Culturing spinal neurons and muscle cells from Xenopus embryos. In Culturing Nerve Cells (ed. G. Banker and K. Goslin), pp. 137-153. The MIT Press, Cambridge, Mass. Tessier-Lavigne, M. and Goodman, C. (1996). The molecular biology of axon guidance. Science 274, 1123-1133. Winkel, G. K. and Nuccitelli, R. (1989). Large ionic currents leave the primitive streak of the 7.5-day mouse embryo. Biol. Bull. 176(S), 110-117. (Accepted 30 September 1997)