Structural Requirements for Outside-In and Inside-Out Signaling by Drosophila Neuroglian, a Member of the L1 Family of Cell Adhesion Molecules

The 1B7 and 3F4 mAbs against Drosophila neuroglian, a rat antiserum specific for the neuroglian¹⁶⁷ protein (Bieber et al., 1989; Hortsch et al., 1995) and affinity-purified rabbit anti-Drosophila ankyrin (Dubreuil and Yu, 1994) have been described earlier. The rat antiserum and the mouse 1D4 mAb against Drosophila fasciclin II, as well as the cDNA for the PEST sequence-containing, transmembrane protein form of Drosophila fasciclin II were kind gifts of C. Goodman (University of California, Berkeley, CA). Rabbit anti-phosphotyrosine antibody (She et al., 1997) was a gift of C. Palfrey (University of Chicago, Chicago, IL). Schneider's medium, penicillin/streptomycin solution, and fetal calf serum were from Life Technologies, Inc. (Gaithersburg, MD).

Cytoplasmic domain deletions were produced by PCR with neuroglian¹⁶⁷ cDNA as template and PCR products were initially subcloned in the pAS-CYH2 vector. 5′ PCR primers used in these PCRs contained a NcoI site (maintaining an open reading frame with the GAL4 DNA-binding domain), followed by a NsiI site; 3′ PCR primers contained a SalI site. The numbers in the designation of individual deletion constructs refer to the 85 amino acid residues of the cytoplasmic domain of the neuroglian¹⁶⁷ protein form. Carboxy-terminal deletions were created by the introduction of in-frame stop codons along the neuroglian sequence using the 3′ PCR primer; deletions in the amino-terminal region of the neuroglian cDNA by using several 5′ PCR primers with homology to different regions of the neuroglian cDNA. The fidelity of the PCR amplification reactions was verified by DNA sequence analysis (Sanger et al., 1977).

Constructs incorporating the cytoplasmic deletions into the complete neuroglian open reading frame were derived from the first set of verified pAS1-CYH2 plasmids. NsiI/SalI cDNA fragments were isolated from the pAS1-CYH2 DNAs and introduced into the context of the entire neuroglian open reading frame by subcloning into pRmHa3:nrg^NsiI vector DNA. This vector was created by using PCR to introduce a silent C to A point mutation at position 3,480 of the neuroglian sequence at the end of the region encoding the transmembrane segment, thereby creating a unique NsiI site.

Neuroglian cDNAs with point mutations converting cytoplasmic tyrosine residues into phenylalanine residues were created using the following strategy. The unique BamHI site at position 3,710 of the neuroglian¹⁶⁷ cDNA sequence was used in a two-step PCR process to create initially single and subsequently double point mutations. This was accomplished by converting the flanking codons encoding tyrosine 1,217 and tyrosine 1,234 into phenylalanine-encoding codons. PCR primers including the BamHI site and one of the Y to F mutated codons (TAT/C to TTT/C) were used in separate PCR reactions and subsequently subcloned into BamHI and either NcoI- or SalI-digested pAS1-CYH2:nrg^wt (construct no. 1, wt) vector DNA. The incorporation of only the desired point mutation(s) was verified by DNA sequence analysis. As described above for the deletion mutations, all three cDNA fragments encoding Y to F mutated, neuroglian¹⁶⁷ cytoplasmic domains were subsequently subcloned into the pRmHa3:nrg^NsiI vector for transfection of S2 cells.

A chimeric cDNA was constructed by the in-frame fusion of DNA fragments encoding the extracellular domain of Drosophila fasciclin II and the transmembrane segment plus the cytoplasmic domain of Drosophila neuroglian¹⁶⁷. A 0.45-kb KpnI/SalI PCR product encoding the neuroglian transmembrane segment and the cytoplasmic domain was derived from a Drosophila neuroglian¹⁶⁷ cDNA and subcloned into pRmHa3 vector DNA. Besides the KpnI cloning site, the 5′ PCR primer also introduced an AatII site which was in-frame with the AatII site at position 2,581 in the fasciclin II cDNA. This interim construct was cut with KpnI and AatII and then ligated to a 2.6-kb fasciclin II cDNA fragment, resulting in the final pRmHa3–fasII^EC–nrg^TM+CP construct. The entire open reading frame of the transmembrane, PEST sequence-containing fasciclin II cDNA, was subcloned into the pRmHa3 vector yielding the pRmHa3–fasII^PEST construct.

All Drosophila S2 cell lines were transfected using Lipofectin^® (Life Technologies, Inc.) and clonal lines were maintained as previously described (Bieber, 1994). After induction with 0.7 mM of CuSO₄, subclones were analyzed by Western blotting for high level expression of recombinant proteins and subclones expressing comparable quantities of neuroglian were selected for further experiments.

The ability of mutated neuroglian to induce homophilic cell aggregation of transfected S2 cells was tested as described earlier (Hortsch et al., 1995). Cell lines were adjusted to a concentration of 10⁶ cells/ml and neuroglian synthesis was induced by the addition of 0.7 mM of CuSO₄. Duplicate cultures (10⁶ cells in 1 ml) were grown in six-well tissue culture plates and induced at 25°C for 15 h. Cells were transferred to sterile 50-ml centrifuge tubes and further incubated on a shaking platform (model 62; New Brunswick Sci. Co., Edison, NJ) at 200 rpm. For a quantitative analysis, the number of nonaggregated cells was counted in a hemocytometer (Bright-Line^®; Reichert, Buffalo, NY). Since cell clusters of up to five cells were occasionally observed in untransfected S2 cells, only aggregates containing more than five cells were considered to be aggregated. Eight fields, each representing 0.01 μl of cell suspension, were counted per culture. Based on the starting number of cells, the results are presented as percent aggregated cells of total cells.

For Western blots, transfected S2 cells were pelleted and solubilized in SDS-containing buffer. Total cell proteins were separated by PAGE, transferred onto nitrocellulose filters, and then probed with specific antibodies as described (Hortsch et al., 1985; Dubreuil et al., 1987). Proteins were separated on either 7.5/0.2% or 8.0/0.08% acrylamide:bisacrylamide gels.

The yeast two-hybrid system was used as described by Durfee et al. (1993). The pACTII–ankyrin construct has been characterized previously (Dubreuil et al., 1996). The pACTII-control plasmid was kindly provided by J. Clemens (University of Michigan, Ann Arbor, MI). Yeast selection plates and media were made and yeast transformations were performed using established protocols (Ausubel et al., 1988). Staining for β-galactosidase expression in yeast cell colonies was assayed using the substrate 5-bromo-4-chloro-3-indolyl-β-d-galactopyranoside as described (Bartel et al., 1993). Quantitative determinations of β-galactosidase expression were done on 4-ml liquid yeast cultures using O-nitrophenyl-β-d-galactoside as substrate (Ausubel et al., 1988).

Immunofluorescence analysis of Drosophila ankyrin distribution in S2 cell aggregates was performed as described previously (Dubreuil et al., 1996). Briefly, cells were attached to alcian blue–coated microscope slides, fixed in 4% paraformaldehyde, permeabilized in 0.1% Triton X-100, and then reacted with antibodies and washed in pH 7.5 Tris-buffered saline containing 5% newborn calf serum.

To determine the cytoplasmic neuroglian subdomains that are involved in ankyrin binding, we engineered a series of neuroglian deletion constructs to test their ability to interact with Drosophila ankyrin (Fig. 1). Deletion breakpoints were selected to isolate several protein segments that are broadly conserved among members of the L1 gene family. It has previously been shown that these conserved regions form functionally and structurally important L1 subdomains, such as the ankyrin-binding site (Davis and Bennett, 1994; Garver et al., 1997; Tuvia et al., 1997).

Since the interaction between the full-size neuroglian cytoplasmic domain and Drosophila ankyrin can be readily detected using the yeast two-hybrid assay system (Dubreuil et al., 1996; Fig. 2), these neuroglian deletion constructs were initially tested for their ability to interact with a Drosophila ankyrin fusion protein in yeast cells. All constructs containing deletions within the amino-terminal 48-amino acid residues of the cytoplasmic domain interacted with ankyrin at or near wild-type levels in yeast cells (Fig. 2). In all constructs missing the 19 most carboxy-terminal amino acid residues, the neuroglian–ankyrin interaction was significantly reduced, although not abolished. With the exception of construct no. 5, all constructs including residues 49–65 of the neuroglian cytoplasmic protein domain exhibited strong binding to the ankyrin fusion protein. Yeast colonies transfected with construct no. 5, which lacks the carboxy-terminal 19-amino acid residues of the neuroglian cytoplasmic domain, developed a weak signal only after prolonged incubation. In contrast, after the same length of incubation no positive signal was ever detected in yeast colonies harboring control pAS-CYH2 plasmids or neuroglian deletion constructs nos. 4, 6, 7, or 8. The smallest region which mediated ankyrin binding at a low level consists of a well conserved 17-amino acid segment (Fig. 1; present in construct no. 3 and absent in construct no. 4). High efficiency binding between the neuroglian and the ankyrin fusion proteins, however, was only observed when the adjacent carboxy-terminal 19-amino acid residues were also present. These results indicate that the conserved FIGQY motif, which was previously shown to be important for ankyrin binding (Davis and Bennett, 1994; Garver et al., 1997), is necessary but not sufficient for high efficiency ankyrin binding. A low-level interaction with ankyrin was still observed for two constructs (nos. 5 and 9) missing this motif.

The same set of cytoplasmic domain deletions was spliced to the remainder of the full-length neuroglian coding sequence for expression studies in Drosophila S2 cells. These recombinant neuroglian cDNA constructs yielded polypeptides with the expected apparent molecular weights in Western blots probed with anti-neuroglian antibodies (data not shown) and they induced robust S2 cell aggregation (Fig. 3,A). A double-label immunofluorescence analysis of the neuroglian and ankyrin distribution in S2 cells indicated that wild-type neuroglian was abundant over the entire cell surface, yet ankyrin was exclusively recruited to sites of cell–cell contact (Dubreuil et al., 1996; Fig. 4 A).

Expression of the Δ18N neuroglian deletion protein (construct no. 2, lacking the 18 amino-terminal residues of the cytoplasmic domain) in S2 cells resulted in the same pattern of ankyrin and neuroglian staining which was observed with wild-type neuroglian (Fig. 4,B). However, none of the other deletion constructs tested (e.g., Δ18N; Δ19C shown in Fig. 4 C) produced any detectable staining of ankyrin at cell contacts or other regions of the cell surface, even though the mutant neuroglian proteins were abundantly expressed at the plasma membrane. Thus, the ankyrin recruitment assay in S2 cells revealed a more complex requirement of the neuroglian cytoplasmic domain in ankyrin binding than was expected based on the results of the yeast two-hybrid assay.

A conserved cytoplasmic tyrosine residue in rat neurofascin, corresponding to Y1234 in neuroglian, was previously shown to have a possible regulatory role, since phosphorylation of this residue inhibited the binding of ankyrin to neurofascin in vitro (Garver et al., 1997). Here the effects of tyrosine to phenylalanine mutations at two positions of the Drosophila neuroglian cytoplasmic domain on ankyrin binding were evaluated using a yeast two-hybrid assay. The residues Y1217 and Y1234 in neuroglian correspond to the tyrosine residues in rat neurofascin which were mutated and analyzed by Garver et al. (1997). Replacement of Y1217 with a phenylalanine had no detectable effect on ankyrin binding (Fig. 5). However, the Y1234F mutation had a significant effect, reducing ankyrin binding by ∼50%. The double mutant Y1217F/Y1234F form reduced ankyrin binding to a similar extent. Thus, the conserved Y1234 contributes to the interaction between ankyrin and neuroglian. However, in contrast to rat neurofascin (Tuvia et al., 1997), substitution of the tyrosine residue with phenylalanine in neuroglian greatly reduced its ability to bind ankyrin.

The same tyrosine mutations (Y1217F and Y1234F) were engineered into the complete neuroglian coding sequence for analysis of ankyrin-binding activity in S2 cells. Aggregates expressing wild-type neuroglian were typically large and cells often exhibited significant neuroglian staining over all regions of the plasma membrane (Fig. 6,A, arrow). In contrast, the most conspicuous ankyrin staining was observed at cell–cell contacts (Fig. 6,A, right). Additional ankyrin staining was visible as a diffuse pattern throughout the cytoplasm and, in many cases, as a punctate pattern in the peripheral cytoplasm. This fainter pattern of ankyrin staining is probably not associated with the plasma membrane since it failed to colocalize with plasma membrane markers such as neuroglian, and it was also visible in the absence of neuroglian expression (Dubreuil et al., 1996). The same patterns of neuroglian and ankyrin staining were observed in cultures expressing the Y1217F mutant form of neuroglian (Fig. 6,B), although the efficiency of ankyrin recruitment was slightly lower than with wild-type neuroglian (Fig. 7). There was a dramatic drop in the efficiency of ankyrin recruitment in cells expressing the Y1234F neuroglian mutation or the double mutant (Fig. 6, C–F, arrowheads). Most contact sites in which neuroglian was prominently stained showed little or no recruitment of ankyrin in cells expressing the Y1234F mutation (e.g., Fig. 6,F). Nevertheless, ankyrin was consistently detected at sites of cell–cell contact in a fraction of cell aggregates expressing these mutations (Fig. 6, C–F and Fig. 7).

Although there was a significant effect of the Y1234F mutation on the efficiency of ankyrin recruitment, there was no apparent effect on the selectivity of recruitment. As with wild type, the only significant colocalization of ankyrin with Y1234F neuroglian occurred at sites of cell contact (Fig. 6, C–E), even though neuroglian was often abundant at noncontact regions of the plasma membrane (e.g., Fig. 6 D, arrow). It should be noted that although the panels shown in the figure were chosen to demonstrate the selectivity of ankyrin recruitment, most of the mutant cell clusters analyzed in the experiment did not exhibit detectable ankyrin staining at cell contacts (Fig. 7). Ankyrin also failed to colocalize with neuroglian in single cells that had not yet joined an aggregate (Fig. 6 G). These results are consistent with the previous observation that ankyrin colocalizes with neuroglian only at sites of cell contact, and not with neuroglian found at noncontact regions of the plasma membrane (Dubreuil et al., 1996). Since cytoplasmic tyrosine mutations did not lead to colocalization of ankyrin with neuroglian at noncontact regions of the plasma membrane, a mechanism other than the phosphorylation of these residues must be responsible for the observed selectivity of ankyrin recruitment.

Further evidence that tyrosine phosphorylation is not responsible for neuroglian regulation in S2 cells was obtained by staining Western blots of neuroglian-expressing S2 cell lysates with a phosphotyrosine-specific antibody (Fig. 8). After induction, neuroglian was readily detected with a neuroglian-specific antibody (Fig. 8, lane 2, left column), but not with the anti-phosphotyrosine antibody (Fig. 8, lane 2, right column). Faint bands in the region of neuroglian were also detected by the anti-phosphotyrosine antibody in uninduced cells (Fig. 8, lane 1, right column) where neuroglian was undetectable (Fig. 8, lane 1, left column). PC12 cells treated with nerve growth factor were used as a positive control. Tyrosine-phosphorylated mitogen-activated protein (MAP) kinase was readily detected in growth factor-induced PC12 cells (Fig. 8, lane 4, **) but not in control untreated cells (Fig. 8, lane 3) (Boulton et al., 1991).

The effect of cytoplasmic mutations on neuroglian-mediated cell adhesion was analyzed in qualitative and quantitative S2 cell aggregation assays. It was previously shown that a glycosyl phosphatidylinositol-linked form of neuroglian lacking the entire cytoplasmic domain nevertheless exhibited robust cell adhesion (Hortsch et al., 1995). All of the neuroglian cytoplasmic domain deletion mutants analyzed here also exhibited strong cell aggregation comparable to cells expressing wild-type neuroglian (refer to Fig. 3,A). In contrast, when analyzing the Y to F mutant neuroglian forms for their competence to recruit ankyrin in S2 cells, we observed that neuroglian molecules harboring a Y1234F mutation consistently induced smaller cell aggregates when compared with wild-type or Y1217F-mutant forms (Fig. 9, A–E). Although a majority of cells expressing wild-type or Y1217F-mutant neuroglian had joined large cell aggregates after 2 h of incubation, cell aggregation was significantly reduced in S2 cell cultures expressing Y1234F-mutant neuroglian (Fig. 9,D). After prolonged incubation times (4–24 h) the mutant neuroglian-expressing cell lines did form somewhat larger aggregates, but never reached wild-type levels (data not shown). This effect was not due to a reduced level of neuroglian protein produced by these cell lines, since Western blot analysis demonstrated similar quantities of neuroglian in induced cultures (Fig. 9 F).

The mechanism behind the adhesion-based neuroglian signal was further examined with a chimeric cDNA composed of the extracellular domain of the Drosophila CAM fasciclin II linked to the cytoplasmic and transmembrane domains of neuroglian. Fasciclin II is also a member of the Ig superfamily, but it is distantly related in sequence and distinct from neuroglian in domain organization (Grenningloh et al., 1991). If the neuroglian signal is simply a consequence of cell adhesion, then the chimera should mimic authentic neuroglian in its ability to induce the recruitment of ankyrin to sites of cell contact. However, if the signal depends on allosteric communication between the extracellular and intracellular domains of neuroglian, then the signal should be uncoupled in the chimeric molecule. The fasciclin II cDNA used here encodes a 115-kD transmembrane protein with a 104-amino acid cytoplasmic domain that is unrelated to neuroglian (Fig. 10). Expression of authentic fasciclin II in S2 cells caused extensive cell aggregation (Fig. 11, A and B), but did not direct ankyrin recruitment to cell contacts (Fig. 11,A). In contrast, expression of the fasciclin II-neuroglian chimera resulted in cell aggregation and recruitment of ankyrin to sites of cell–cell contact (Fig. 11, C and E). Ankyrin was not recruited to nonadherent regions of the plasma membrane in cell aggregates or to the plasma membrane in single cells expressing the chimaera (data not shown). The fasciclin II staining pattern appeared concentrated at sites of cell–cell contact in detergent-permeabilized cells (Fig. 11, B and D). However, control experiments with nonpermeabilized cells revealed that the chimaera was also abundant at nonadherent regions of the plasma membrane (Fig. 11 D, inset). Thus, ankyrin recruitment coincided with sites of cell adhesion and not with the total distribution of the chimeric molecule. These results indicate that cell adhesion is a sufficient signal to activate recruitment of ankyrin by the cytoplasmic domain of neuroglian.

In addition to their primary roles in cell adhesion, adhesion molecules from the integrin and cadherin families transduce signals across the plasma membrane (Clark and Brugge, 1995; Gumbiner, 1995). Here we show that neuroglian, a CAM from the Ig superfamily, also has the ability to transduce signals in both directions across the plasma membrane. First, we have investigated the structural requirements for outside-in signaling which leads to selective binding of ankyrin to neuroglian at sites of cell contact. Studies of a fasciclin II-neuroglian chimera revealed that adhesion, rather than any unique property of neuroglian's extracellular domain, activates ankyrin binding to the intracellular domain. Phosphorylation of a conserved cytoplasmic tyrosine residue, which was recently shown to inhibit ankyrin binding to a vertebrate neuroglian homologue, neurofascin (Garver et al., 1997; Tuvia et al., 1997), did not regulate ankyrin binding to neuroglian in S2 cells. Second, the extracellular adhesive activity of neuroglian was found to be regulated by the state of the cytoplasmic domain. Although the biological significance of this level of regulation is not yet known, it provides a simple mechanism for the spatial and temporal regulation of L1 family members. These observations broaden our understanding of how extracellular adhesion directs rearrangement of the spectrin/ankyrin membrane skeleton within the cell and how protein interactions inside the cell can regulate extracellular adhesion.

Whereas the inside-out regulation of neuroglian's adhesive function is one finding of the present study, our approach has largely been directed toward the mechanism of outside-in signaling. Drosophila S2 cells provide a unique model system in which to study the recruitment of ankyrin to the plasma membrane, since ankyrin is not ordinarily associated with the plasma membrane of these cells. We previously demonstrated that both Drosophila neuroglian (Dubreuil et al., 1996) and human L1-CAM (Vallejo et al., 1997; Hortsch et al., 1998) induce the selective recruitment of ankyrin to sites of cell contact, even though the adhesion molecules themselves are broadly expressed over the entire cell surface. Once neuroglian has interacted with ankyrin at cell–cell contact sites, it becomes resistant to extraction by nonionic detergents (Dubreuil et al., 1996). This change in the solubility of neuroglian precludes an analysis of the neuroglian–ankryin interaction by immunoprecipitation techniques and, when using immunofluorescence microscopy, results in an underrepresentation of neuroglian staining at noncontact areas of the S2 plasma membrane.

It was previously shown that the FIGQY sequence, which is highly conserved throughout the L1 family, provides an essential part of the ankyrin-binding domain in rat neurofascin (Davis and Bennett, 1994; Garver et al., 1997). Through a combination of yeast two-hybrid analysis and expression of mutated neuroglian molecules in S2 cells, we have mapped a larger, 36-amino acid segment in the neuroglian cytoplasmic domain, which includes this conserved motif, that is both necessary and sufficient to allow the interaction between neuroglian and ankyrin.

The demonstration that ankyrin binding to rat neurofascin can be regulated by phosphorylation of the tyrosine residue in the FIGQY motif (Garver et al., 1997; Tuvia et al., 1997) suggested a possible mechanism to explain outside-in regulation of neuroglian. Phosphorylation of this conserved tyrosine in the cytoplasmic domain of neurofascin caused an ∼40% reduction in ankyrin binding and a comparable decrease in cell aggregation. Based on these properties of neurofascin, we hypothesized that the association of ankyrin with neuroglian in S2 cells could also be regulated by tyrosine phosphorylation, assuming that the phosphorylation of the tyrosine residue in the FIGQY motif is regulated by cell adhesion.

If neuroglian were phosphorylated on tyrosine residues in S2 cells, and phosphorylation was responsible for the lack of ankyrin binding to neuroglian at noncontact sites of aggregated S2 cells, then the mutation of tyrosine residue 1234 in Drosophila neuroglian would be expected to cause ankyrin binding indiscriminately at all regions of the plasma membrane. Although the neuroglian Y1234F mutation greatly reduced the extent of ankyrin binding to neuroglian, it did not affect the selective association of ankyrin at sites of cell–cell contact or the lack of ankyrin at noncontact regions of the plasma membrane. Thus, another mechanism must be responsible for the outside-in regulation of ankyrin recruitment in S2 cells. We therefore suggest that the previously observed effects of tyrosine phosphorylation on rat neurofascin constitutes a mechanism of regulation that might be specific for the neurofascin subfamily. Alternatively, tyrosine phosphorylation may operate in regulating ankyrin binding to L1 molecules in some cell types, such as the B104 neuroblastoma cell line, but not in other cells. S2 cells may simply lack a tyrosine kinase of the appropriate specificity for the FIGOY motif to produce an effect on ankyrin binding. It is important to note that these two mechanisms for regulating the interaction between ankyrin and L1 molecules are not mutually exclusive, and the phosphorylation of the conserved tyrosine residue in the FIGQY motif might provide an additional way to inhibit L1-mediated cell adhesion and L1 binding to the membrane skeleton.

Other types of protein phosphorylation might also be involved in regulating the association of ankyrin with neuroglian in vivo or in S2 cells. Several cytoplasmic serine residues are also highly conserved throughout the L1 family and some have been shown to be the target of protein kinases (Wong et al., 1996a,b). The phosphorylation of these residues might have an effect on ankyrin binding to L1 family members and play an important role in the regulation of this interaction in S2 cells.

The regulation of ankyrin binding to L1-type molecules might also involve the adhesion-induced clustering of several L1 molecules within the plane of the plasma membrane, similar to the mechanism of growth factor receptor activation (Schlessinger and Ullrich, 1992). Alternatively, the homophilic adhesion process could induce an allosteric change in the neuroglian molecule. However, the finding that a chimeric molecule, composed of the extracellular domain of a distantly related adhesion molecule coupled to the cytoplasmic and transmembrane domains of neuroglian, exhibits the same regulated association with ankyrin as wild-type neuroglian argues against the allosteric model.

Our results indicate that the tyrosine residue in the conserved FIGQY motif plays an important role in L1's interaction with the membrane skeleton and its adhesive function. One of the identified L1-CAM mutations, which causes a range of neurological phenotypes in humans, results in the exchange of tyrosine 1229 in the human L1 protein for a histidine residue (Van Camp et al., 1996). Residue Y1229 in human L1-CAM is homologous to Y1234 in the Drosophila neuroglian sequence. Considering that the cytoplasmic domain of human L1 CAM is dispensable for its adhesive function (Wong et al., 1995a), it has been an enigma why mutations in the cytoplasmic domain of human L1-CAM can cause the same range of phenotypes as mutations in the extracellular domain. It now appears that extracellular adhesive and intracellular cytoskeletal interactions of L1 molecules are functionally connected and therefore influence each other. Members of the L1 family are expressed on advancing growth cones during development and during regeneration after nerve injury and by other motile neuronal cells, such as migrating granule cells (Lindner et al., 1983; Kamiguchi and Lemmon, 1997). A precise regulation of neuronal adhesiveness must be very important in these cells to allow dynamic interactions with their cellular environment. Any mutation interrupting this delicate adhesive balance might therefore cause the observed wide range of L1 mutant phenotypes (Wong et al., 1995b; Dahme et al., 1997; Hall and Bieber, 1997).

We would like to thank C. Goodman (University of California, Berkeley, CA) for making the fasciclin II cDNA and the anti-fasciclin II antibodies available to us, C. Palfrey for providing the anti-phosphotyrosine antibody, and M. Wert (both from University of Chicago, Chicago, IL) for PC12 cell samples. We would also like to thank M. Wyche (Alabama A & M University, Normal, AL) and M. Hadeed for help with several of the described experiments and S. Brown and S. Ernst (all three from University of Michigan, Ann Arbor, MI) for a critical reading of the manuscript.

CAM

cell adhesion molecule