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The Journal of Neuroscience, October 25, 2006, 26(43):11120-11130; doi:10.1523/JNEUROSCI.3264-06.2006

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Development/Plasticity/Repair
Olfactory Ensheathing Cells Do Not Exhibit Unique Migratory or Axonal Growth-Promoting Properties after Spinal Cord Injury

Paul Lu,^1,2 Hong Yang,¹ Maya Culbertson,¹ Lori Graham,¹ A. Jane Roskams,³ and Mark H. Tuszynski^1,2

¹Department of Neuroscience, University of California at San Diego, La Jolla, California 92093, ²Veterans Affairs Medical Center, San Diego, California 92161, and ³Department of Zoology, University of British Columbia, Vancouver, British Columbia, Canada V6T 1Z4

	Abstract

Top Abstract Introduction Materials and Methods Results Discussion References

 
Olfactory ensheathing cells (OECs) have been reported to migrate long distances and to bridge lesion sites, guiding axonal regeneration after spinal cord injury (SCI). To understand mechanisms of OEC migration and axonal guidance, we injected lamina propria OECs 1 mm rostral and caudal to C4 SCI sites. One month later, OECs formed an apparent migrating cell tract continuously extending from the injection site through the lesion, physically bridging the lesion. Confocal immunolabeling demonstrated that, whereas this cell tract displaced host astrocytes, descending or ascending long tract axons did not preferentially extend into the cell tract and OECs failed to support bridging of corticospinal axons. Notably, the "bridging" tract of OECs formed within 1 h of cell injection, raising the possibility that cells passively spread from the pressure injection site rather than actively migrating. Control injections of bone marrow stromal cells (MSCs) or fibroblasts 1 mm from the lesion site also rapidly dispersed into the lesion cavity. Cell tracts extending into the lesion site were not seen when cells were injected either at low volumes, into spinal cord gray matter, or 3 d before or 9 d after SCI. OECs proliferated in injection sites, cell tracts, and lesion sites, indicating that OECs can also accumulate through cell proliferation. Thus, OECs do not appear to exhibit significant migratory properties when grafted to the spinal cord, exhibit no detectable difference in promoting axon growth into a SCI site compared with MSCs or fibroblasts, and do not support bridging of corticospinal axons beyond a dorsal column lesion.

Key words: olfactory ensheathing cells; spinal cord injury; migration; axon growth; axon guidance; proliferation

	Introduction

Top Abstract Introduction Materials and Methods Results Discussion References

 
Olfactory ensheathing cells (OECs) are glial cells that ensheath the axons of olfactory receptor neurons extending from the olfactory epithelium to the olfactory bulb (Doucette, 1995; Chuah and West, 2002). OECs have been reported to guide and support the entry and growth of axons from newly born olfactory receptor neurons to their target CNS tissue after transection of the olfactory nerve (Graziadei and Monti Graziadei, 1980; Doucette et al., 1983; Doucette, 1990). Because of these proposed axon growth-promoting properties, OECs have been extensively studied and transplanted into the injured spinal cord or the dorsal root entry zone in an attempt to promote axonal regeneration (Ramon-Cueto and Nieto-Sampedro, 1994; Li et al., 1997, 1998, 2004; Ramon-Cueto et al., 1998, 2000; Navarro et al., 1999; Imaizumi et al., 2000a,b; Boruch et al., 2001; J. Lu et al., 2001, 2002; Nash et al., 2002; Pascual et al., 2002; Ruitenberg et al., 2002, 2003, 2005; Takami et al., 2002; Gomez et al., 2003; Keyvan-Fouladi et al., 2003; Plant et al., 2003; Resnick et al., 2003; Verdu et al., 2003; Andrews and Stelzner, 2004; Boyd et al., 2004; Cao et al., 2004; Chuah et al., 2004; Garcia-Alias et al., 2004; Lee et al., 2004; Lopez-Vales et al., 2004, 2006; Pearse et al., 2004; Polentes et al., 2004; Ramer et al., 2004a,b; Riddell et al., 2004; Sasaki et al., 2004; Barakat et al., 2005; Collazos-Castro et al., 2005; Fouad et al., 2005; Richter et al., 2005; Moreno-Flores et al., 2006). Many of the above studies report that OECs promote axonal regeneration and, in some cases, functional recovery, although controversy exists (Gomez et al., 2003; Ramer et al., 2004b; Riddell et al., 2004; Steward et al., 2006). Nonetheless, cells referred to as OECs have recently been implanted into 1000 human patients with spinal cord injury (Huang et al., 2003; Dobkin et al., 2006).

Initial studies hypothesized that migratory properties of OECs account in part for their "repair" qualities, because OECs were found to migrate and associate with extending axons in the lesioned spinal cord (Ramon-Cueto and Nieto-Sampedro, 1994; Li et al., 1997, 1998; Ramon-Cueto et al., 1998, 2000; Boruch et al., 2001). For example, in some studies, OECs were injected 1 mm rostral and caudal to a lesion site, and it was reported that OECs migrated longitudinally as far as 1.5 cm from the host/lesion interface (Ramon-Cueto et al., 1998). Furthermore, colocalization of migrating OECs and regenerating corticospinal and serotonergic axons was proposed to provide permissive conditions for axon bridging beyond the lesion site (Ramon-Cueto et al., 1998, 2000).

The present study originally sought to identify molecular mechanisms potentially underlying migratory properties of OECs. Well characterized OECs derived from lamina propria were genetically modified to express the reporter gene green fluorescent protein (GFP) to enhance tracking into sites of mid-cervical spinal cord injury (Au and Roskams, 2002, 2003; Ramer et al., 2004a). Unexpectedly, we failed to find unique migratory properties of these cells when implanted into spinal cord lesion sites, and we further find that grafted tracts of cells tend to displace established spinal pathways rather than exhibiting unique axon growth-promoting properties.

	Materials and Methods

Top Abstract Introduction Materials and Methods Results Discussion References

 
Cell culture. Lamina propria OECs were harvested from the olfactory mucosa of postnatal day 5 Fischer 344 rats, as described previously (Au and Roskams, 2003; Ramer et al., 2004a). Briefly, the entire olfactory mucosa, including turbinates and septum, was dissected from 8–10 pups, mechanically dissociated and digested using 0.6 mg/ml Collagenase D (Roche, Welwyn Garden City, UK), 3 U/ml dispase I (Roche), 15 µg/ml hyaluronidase (Sigma, St. Louis, MO), 0.5 mg/ml bovine serum albumin (MP Biomedicals, Irvine, CA), and 100 U/ml DNase I (Sigma) for 1 h at 37°C, before centrifugation and plating. Initial plating in MEM-D-Valine (Invitrogen/BRL, Eugene, OR), 10% fetal bovine serum (FBS), and 100 U/ml penicillin/streptomycin (P/S) (Invitrogen/BRL) was followed 4–5 d later by purification using anti-Thy 1.1-mediated complement lysis to remove contaminating fibroblasts. Cells were replated in DMEM/F12 (Invitrogen/BRL), 10% FBS, and 100U/ml P/S, allowed to grow for an additional 4–6 d, and were again subjected to Thy1.1-mediated complement lysis.

Primary rat bone marrow stromal cells (MSCs) were isolated according to the method of Azizi et al. (1998). Briefly, the tibias and femurs of adult female Fischer 344 rats (3 months old, 150–165 g) were dissected. The ends of the bone were cut and 5 ml of DMEM (Invitrogen/BRL) cell culture medium were injected into the central canal of the bone to extrude the marrow. Whole marrow cells were cultured at a density of 5–10 x 10⁵ cells/cm² in -MEM medium (Invitrogen/BRL) supplemented with 20% FBS and P/S. After 24 h, nonadherent cells were removed and the medium was changed every other day until cells became confluent.

Primary cultures of rat fibroblasts were generated from skin biopsies of adult female Fischer 344 rats as described previously (Tuszynski et al., 1996) and maintained in standard medium (DMEM with high glucose; Invitrogen/BRL) containing 10% fetal bovine serum and penicillin/streptomycin.

Transduction of primary cells with the GFP reporter gene. To monitor grafted cell migration in vivo, primary OECs, MSCs, and fibroblasts were transduced with the jellyfish GFP reporter gene as described previously (Lu et al., 2005). Briefly, the retroviral vector plasmid DNA pLXSN-GFP was transfected into the stable viral producer line PA317 using the ecotropic packaging cell line psi-2, as described previously (Tuszynski et al., 1996). The virus collected from 24 h conditioned medium was used to infect either primary OECs, MSCs, or fibroblasts at early passage (p1–p2). GFP-expressing OECs and MSCs were analyzed and sorted following standard procedures by a fluorescent-activated cell sorting scan directed to detection of GFP fluorescence, with a standard excitation wavelength of 488 nm. GFP-expressing fibroblasts were purified by G418 selection as described previously (Tuszynski et al., 1996).

Assessment of OEC purity. To assess purity of OECs before transplantation, small aliquots of cells at passage 6 were seeded into 24-well plates for 24 h then fixed in 4% paraformaldehyde for p75 low affinity neurotrophin receptor immunocytochemical labeling (see below, histology and immunocytochemistry) (Au and Roskams, 2003; Jani and Raisman, 2004). The number of p75 and GFP double-labeled cells was then quantified in five randomly selected fields at 400x under a fluorescence microscope, and divided by the total number of GFP-expressing OECs in that field, to obtain the mean percentage of cells expressing p75.

Preparation of cells for transplantation. GFP-expressing OECs, MSCs, and fibroblasts at passages 5–7 were harvested with 0.25% trypsin/1% EDTA when they reached 80–90% confluence. Cell suspensions were prepared at a concentration of 100,000 OECs/µl, 75,000 MSCs/µl, and 75,000 fibroblasts/µl in sterile PBS (Invitrogen) and maintained on ice for transplantation.

Surgery. A total of 66 adult female Fischer 344 rats (160–200 g) were subjects of this study. National Institutes of Health (NIH) guidelines for laboratory animal care and safety were strictly followed. Animals had access to food and water ad libitum throughout the study. All surgery was done under anesthesia with a combination (2 ml/kg) of ketamine (25 mg/ml), rompun (1.3 g/ml), and acepromazine (0.25 mg/ml).

A previously characterized cervical spinal cord dorsal column wire-knife lesion model (Weidner et al., 2001; Lu et al., 2004, 2005) was used for this study. Briefly, a Kopf microwire knife (Kopf Instruments, Tujunga, CA) was stereotaxically positioned at the C4 spinal dorsal midline, then moved 0.6 mm left laterally and lowered 1.1 mm from the dorsal spinal cord surface. The knife blade was extruded 2.25 mm toward the midline, forming a 1.5 mm wide wire arc. The arc was raised 2 mm and was simultaneously met by a blunt glass rod that added compression from above to ensure full transection of axons in the dorsal columns bilaterally.

Immediately after completing the lesion, 0.75 µl of OECs were stereotaxically microinjected into the spinal cord dorsal column midline, 1 mm rostral and 1 mm caudal to the wire-knife lesion site, at a depth of 0.75 mm using a pulled glass micropipette with an inner diameter of 40 µm, connected to a Picospritzer II (General Valve, Fairfield, NJ). The cells were injected at a rate of 200 nl/min. This injection delivered cells into dorsal column white matter near the interface with spinal gray matter (eight injections in four subjects killed 1 month after cell injection). Comparison was also made to subjects that received direct OEC injections in the acute lesion cavity (injections into lesion sites in four animals killed 1 month after cell injection; volume 1.5 µl cells/lesion site).

After obtaining early experimental results (see Results), we added several control groups to further assess cell injection paradigms in this experiment. To control for the possibility that pressure cell injections might permit cells to track down a pathway of least resistance at the interface of white and gray matter toward the lesion site, or through diminished resistance along tracts of white matter, one control group received injections of OECs confined entirely within dorsal gray matter, 0.8 mm lateral to midline, 0.6 mm ventral to the dorsal spinal cord surface, and 1 mm rostral and caudal to the lesion site (four injections in two subjects). To further address the possibility that injection under pressure might cause cells to rapidly diffuse down a path of least resistance toward the lesion site rather than migrate at slower rates over time, the time course of OEC distribution from the site of injection toward the lesion cavity was examined; 0.75 µl of OECs were injected in the dorsal column midline at a depth of 0.75 mm, 1 mm rostral and 1 mm caudal to the lesion site, and subjects were perfused at time points of 1, 3, 12, and 24 h, 3 d, and 7 d postinjection (four injections in two subjects at each time point). To provide an additional control for the possibility that cell injection under pressure favored passive cell diffusion down a low-pressure gradient, a very small volume of cells (50 nl) was slowly injected over 5 min into the dorsal white matter midline at a depth of 0.75 mm, at a distance 1 mm rostral and 1 mm caudal to the lesion site (12 injections in six subjects).

To further control for the possibility that OECs diffused rapidly down a low-pressure gradient that existed immediately after lesion placement, 0.75 µl of OECs were injected either 3 d before lesion placement (before a low pressure gradient could exist), or 9 d postlesion (a time point at which an acute lesion-related low-pressure gradient would resolve). Cells were injected into the dorsal column midline at a depth of 0.75 mm, and a distance 1 mm rostral and 1 mm caudal (eight injections in four subjects at each time point).

To address the possibility that OECs respond to migratory signals acting over a distance, OECs were injected at greater distances from the lesion site: 0.75 µl of OECs were injected 3 mm rostral and 3 mm caudal to the lesion site, in the spinal cord midline at a depth of 0.75 mm (four injections in two subjects). OECs were also injected into the dorsal column white matter of intact animals to examine cell distribution in the noninjured environment (injections at the C4 level, spaced 2 mm apart in the rostral–caudal dimension, and injected into the dorsal column midline at a depth of 0.75 mm; four injections in two subjects).

Finally, to determine whether either cell migration or passive cell diffusion from the injection site was a characteristic unique to OECs, additional animals received injections of either bone marrow stromal cells (MSCs) or fibroblasts using the same paradigm used for OEC injections. Subjects underwent C4 dorsal column wire knife lesions and received injections of 0.75 µl of MSCs or fibroblasts into the midline dorsal columns at a depth of 0.75 mm, at a distance 1 mm rostral and 1 mm caudal to the lesion site (n = 4 injections in two subjects per condition per time point). Subjects were killed 1, 3, 12, and 24 h, 3 d, and 7 d postinjection for MSCs, or 1 h, 3 h, and 3 d postinjection for fibroblasts.

Unless stated otherwise, subjects were killed 7 d after cell injection.

To examine proliferation of grafted OECs in vivo, bromodeoxyuridine (BrdU; Sigma) was injected intraperioneally daily, 40 mg/kg in sterile saline, for five consecutive days beginning 1 d postlesion. BrdU was injected intraperitoneally in four subjects that received OEC implants into dorsal column white matter, 1 mm rostral and 1 mm caudal to the lesion site, at a depth of 0.75 mm. Subjects were killed 1 week after lesion placement.

In subjects that received OEC injections into dorsal white matter immediately after spinal cord lesions, the corticospinal tract (CST) was anterogradely labeled using biotinylated dextran amine (BDA, MW 10,000; Invitrogen). Subjects received BDA injections 2 weeks before killing, and survived a total of 1 month postlesion. A total of 100 nl of a 10% solution of BDA dissolved in H₂O was injected into each of 18 sites spanning the rostral-to-caudal extent of the motor cortex with a Picospritzer (General Valve), using methods and injection coordinates reported previously (Lu et al., 2005). Ascending dorsal column sensory axons were transganglionically labeled with cholera toxin B subunit (CTB; List Biologic, Campbell, CA) injected into both sciatic nerves 3 d before perfusion, as described previously (Lu et al., 2005).

Histology and immunocytochemistry. At the end of each survival period, subjects were perfused with 4% paraformaldehyde in 0.1 M phosphate buffer, pH 7.4. Spinal cords were dissected, postfixed overnight at 4°C and transferred to 30% sucrose for 72 h. Sagittal sections of spinal cords from the cervical lesion site were cut on a cryostat set at 30 µm thickness, and one of every seven sections was mounted on gelatin-coated slides for Nissl staining. The remaining sections were serially collected into 24-well plates for immunocytochemistry.

Double or triple fluorescent immunocytochemistry was performed to assess cultured and grafted OEC purity, grafted OEC location, and migration at various survival times. After blocking nonspecific antibody reactions with 5% donkey serum for 1 h at room temperature, free-floating sections were incubated with primary antibodies directed against jellyfish GFP [polyclonal (rabbit or goat) antibody from Invitrogen at 1:1,500 to label GFP transduced OECs, MSCs, and fibroblasts], p75 [polyclonal (rabbit) antibody from Sigma at 1:100 to determine purity of OECs], GFAP [monoclonal antibody from Chemicon (Temecula, CA) at 1:1,000 to label host tissue astrocytes], neurofilament (NF; RT97 monoclonal antibody from Chemicon at 1:3,000 to label host tissue axons), serotonin (5-HT; monoclonal antibody from Chemicon at 1:15,000 to label raphespinal axons), CTB [polyclonal (goat) antibody from List Biologic at 1:5,000 to label dorsal column sensory axons], BrdU (monoclonal antibody from Chemicon at 1: 400 to label dividing cells), and Alexa 594-conjugated streptavidin (to bind to BDA-labeled corticospinal tract axons) overnight at 4°C. After washes, sections were incubated either with Alexa 488, Alexa 594- or Cy5-conjugated donkey anti-mouse, donkey anti-rabbit, or donkey anti-goat secondary antibodies (1:150; Invitrogen) or biotinylated donkey anti-rabbit secondary antibody (for p75 labeling, 1:150; Vector Laboratories, Burlingame, CA) for 2.5 h at room temperature. After incubation with biotinylated secondary antibody, sections were incubated with streptavidian Alexa 594 (1:300; Invitrogen) at room temperature for another 2.5 h. The sections were then washed, mounted on uncoated slides and coverslipped with Fluoromount G (Southern Biotechnology, Birmingham, AL).

Quantification of axon density within spinal cord lesion/graft site or within cell migration tract and host tissue. The density of NF-labeled axons penetrating spinal cord lesion/graft sites, or within cell tracts and adjacent host tissue, was quantified using NIH Image software analysis of immunolabeled sections, as described previously (Tuszynski et al., 1996). The margins of the lesion were determined from outlines of GFAP immunolabeling. Alexa594 fluorescent images of NF-labeled axons from two randomly selected parasagittal sections from each animal were captured using an Olympus (Tokyo, Japan) confocal microscope and a sample box size of 512 x 512 pixels, under a 10x objective. Images were converted into black and white using NIH Image software, and the number of pixels occupied by NF-labeled axons within (1) each cell tract, (2) the lesion/graft site, or (3) the surrounding host spinal cord parenchyma surrounding each "migrating" cell tract was measured and divided by sample area to obtain mean NF-labeled axon density per pixel. Comparison was made to subjects that received implants of either GFP-expressing MSCs or GFP-expressing fibroblasts into the lesion site, in sections taken from previous studies (P. Lu et al., 2001; Lu et al., 2005) (n = 4 animals per group surviving 1 month). Results are expressed as axon density per pixel ± SEM.

GFP-expressing OECs that colocalized with BrdU were quantified in four subjects surviving for 1 week after grafting into midline dorsal column white matter (0.75 mm depth). Two randomly selected Z-stack optical section images were acquired under a 60x high numerical aperture oil objective in each of five regions (rostral injection site, rostral cell tract, lesion site, caudal cell tract, and caudal injection site) in each subject, using an Olympus FluoView 1000 confocal microscope (see Fig. 9). GFP/BrdU double-labeling of cells was determined from Z-stack images using Volocity software (Improvision, Coventry, UK) after three-dimensional reconstruction, and was expressed as the percentage of total GFP-labeled cells that colocalized with BrdU (i.e., the percentage of dividing OECs).

Statistical analysis. In all quantification procedures, observers were blinded to the nature of the experimental manipulation. Multiple group comparisons were made using one-way ANOVA and a designated significance level of 95%. Post hoc differences were tested by Fischer's least square difference. Data are presented as mean ± SEM.

	Results

Top Abstract Introduction Materials and Methods Results Discussion References

 
OECs survive and extend in a cell tract toward the lesion site after rostrocaudal transplantation
P75 immunocytochemical labeling revealed that 97.6 ± 0.4% of GFP-expressing OECs labeled for p75 before in vivo grafting (Fig. 1A–C). After transplantation 1 mm rostral and caudal to the C4 spinal cord injury site, OECs survived at all time points examined and expressed both GFP and p75 (Fig. 1D–E). Grafted MSCs and fibroblasts, and sections in which primary antibody was omitted, did not label for p75 (data not shown).

View larger version (113K): [in this window] [in a new window]   Figure 1. p75 immunolabeling of GFP-expressing OECs in vitro and in vivo. A–C, After passage 6, the majority of GFP-transduced OECs (A; green) express p75 (B, red; C, yellow). D, Double florescent immunolabeling shows that the majority of GFP-expressing OECs express p75, 7 d after transplantation. E, xy, xz, and yx plane images of a typical GFP and p75 double-labeled OEC taken from the central field of D. Scale bars: A–C, 35 µm; D, 63 µm; E, 10 µm.

 
We reported previously that wire-knife lesions transect the cervical dorsal columns, including dorsal column sensory axons and dorsal corticospinal tract axons, and that cystic cavities form if cells are not transplanted (Weidner et al., 2001; Lu et al., 2003, 2004, 2005). After injection of OECs 1 mm rostral and 1 mm caudal to the lesion site immediately after placement of lesions, OECs readily survived and formed a continuous tract of cells extending from injection sites to completely fill the lesion cavities, assessed 1 month postlesion and grafting (Figs. 2–5). The apparent number and density of cells occupying the lesion site appeared greatest in subjects that received OEC implants rostral and caudal to the lesion site, rather than direct OEC injections into the lesion site, as reported previously (Fig. 2) (Richter et al., 2005). The size of the lesion cavity did not differ between animals receiving rostral/caudal cell injections or injections directly into the lesion site (Figs. 2–5).

View larger version (162K): [in this window] [in a new window]   Figure 2. OEC injection 1 mm from lesion site. A, Nissl-stained section demonstrating the morphology of rostral and caudal OEC injection sites (IS; arrowhead) and lesion site (Les; outlined by dashed lines). B–C, Higher magnification of boxed areas in A, showing filling of lesion site with OECs injected 1 mm distantly (B), and a cell tract (Tract; arrow) extending caudally from the injection site (IS; C). D, Graft/lesion morphology in a control subject wherein OECs were directly injected into lesion site (outlined by dashed lines). g, Graft; h, host. E, Higher magnification of lesion area in D. Cells injected 1 mm away from the lesion site (B) reconstitute a more regular cellular matrix than cells directly injected into lesion site (E). Scale bars: A, 380 µm; (in E) B, C, E, 42 µm; D, 208 µm.

 

View larger version (113K): [in this window] [in a new window]   Figure 3. OEC Tract formation and relationship to corticospinal axons. A, Triple fluorescent immunolabeling for injected OECs (green; expressing GFP), host astrocytes (GFAP; blue) and corticospinal tract axons (red). OECs injected 1 mm rostral to the lesion site form a cell tract extending from injection site (IS) to lesion (Les), 4 weeks after injection. B–D, Higher magnification of confocal Z-stacks from left box in A indicates that parenchymal regions containing injected OECs (green) exhibit reduced labeling for corticospinal axons (red) compared with regions outside the OEC tract (e.g., region within dashed lines). Corticospinal axons are present outside main labeled OEC tract (D, arrowheads). E–H, Higher magnification of middle box in A. Corticospinal axons are not visible within OEC tract extending toward lesion cavity. In addition, GFAP labeling does not colocalize with the tract composed of longitudinally oriented OECs, suggesting that OECs may displace host glia. I, J, Higher magnification of right box in A shows no corticospinal axons (red) growing into and beyond the lesion site containing OECs (green). Scale bars: A, 260 µm; B–J, 35 µm.

 

View larger version (73K): [in this window] [in a new window]   Figure 4. OEC tract formation and relationship to dorsal column sensory axons. A, OECs injected 1 mm caudal to the lesion (Les) also form a cell tract (tract) extending continuously from the injection site (IS) into the lesion. However, CTB-labeled axons (red) penetrate the lesion region not along tracts defined by OEC cells, but directly across the dorsal host/graft interface (arrow). B, Higher magnification of confocal Z-stacks demonstrates CTB-labeled sensory axons in lesion site (arrowheads), independent of OECs. Scale bars: A, 140 µm; B, 45 µm.

 

View larger version (136K): [in this window] [in a new window]   Figure 5. OEC tract formation and relationship to axons. A–E, GFP and NF double fluorescent immunolabeling. A, GFP-expressing OECs (green) form a tract extending continuously between the rostral injection site (IS) and the lesion (Les). B, Higher magnification of A shows that some NF-expressing axons (red) penetrate the lesion site from region of OEC tract, whereas other axons penetrate the lesion independent of OEC tract. C–E, Higher magnification of boxed area in A suggests that NF axon density is lower in OEC tract than surrounding tissue. F, Quantification of neurofilament axon density in OEC cell tracts (R, rostral; C, caudal) and in lesion site (D, direct injection). Axon density in lesion/graft site does not differ among animals transplanted with OECs, marrow stromal cells or fibroblasts. ***p < 0.0001. G, 5HT-labeled raphespinal axons (green) are not observed within OEC tracts or lesion site (Les). Scale bars: A, 140 µm; B–E, G, 32 µm. Error bars indicate SEM.

 
The OEC tract displaces host axons and astrocytes, and does not appear to guide axons toward the lesion site
To address whether rostrocaudally transplanted OECs promote axon growth and regeneration into and beyond the lesion site, we labeled corticospinal axons with BDA and sensory axons with CTB. Corticospinal tract axons did not penetrate grafts in the lesion site (Fig. 3) and were never observed bridging beyond the caudal host–graft interface. Furthermore, corticospinal axons rostral to the lesion site did not exhibit an evident topographical association with GFP-labeled OECs on thin plane confocal images (Fig. 3). Occasional sensory axons penetrated the lesion/graft site (Fig. 4). However, CTB-labeled sensory axons did not preferentially extend along the OEC tract, which was located more ventrally than the rostrally projecting dorsal column sensory axons (Fig. 4). OEC tracts did not contain GFAP-labeled astrocyte cell bodies or processes (Fig. 3).

Tracts of OECs contained a significantly lower mean density of NF-labeled axons compared with the adjacent spinal cord (p < 0.0001) (Fig. 5). Axons extended into lesion sites filled with OECs, indicating that OECs, like other cell types, can constitute a cellular matrix supportive of axon growth into a lesion site (Fig. 5). Nevertheless, the density of axons within the lesion site in rostrocaudally transplanted subjects, in subjects receiving OEC injection directly into the lesion center, and in subjects receiving implants of MSCs or fibroblasts, was similar (Fig. 5). Raphespinal axons (5-HT immunolabeled) were present neither in the linear OEC tract nor within lesion sites (Fig. 5), within the limits of sensitivity of fluorescent immunolabeling used in this experiment.

Time course of OEC distribution in tracts extending toward the lesion site
Given the striking formation of OEC tracts extending from injection to lesion sites 1 month after acute cell injections 1 mm rostral and 1 mm caudal to the lesion site, we examined a set of temporal, spatial, and cellular controls to elucidate mechanisms underlying this apparent migratory behavior. Notably, the arrangement of injected OECs into a linear tract extending from the injection site to the lesion site was present 1 h after lesion/injection in both rostral and caudal directions (Fig. 6). In subjects killed 3 h after OEC injection, more OECs were present in the lesion center, suggesting improved attachment of cells to the lesion cavity or ongoing shifts of OECs from injection sites to the lesion cavity via the cell tracts (Fig. 6). OECs remained small round and compact in the injection sites, cell tracts and lesion site (Fig. 6). By 12–24 h after cell injection, OECs were distributed more dorsoventrally within the lesion cavity (Fig. 6). In addition, OECs extended processes and reassumed more typical streaming (fibroblast-like) morphology. At these stages, the margins of the lesion site expanded in the rostrocaudal direction compared with very early time points postinjection as described previously (Fitch et al., 1999). By 3–7 d after cell injection, OECs almost filled the lesion cavity and cellular morphology became more compact, similar to the appearance of OECs remaining with injection sites and cell tracts (Fig. 6). Although OEC processes were randomly oriented within the lesion and injection site, cells were rostrocaudally oriented in the tracts leading to the lesion site. Rare OECs could be observed up to distances of 100 µm outside the region of cell injection sites and tracts at time points of 3–7 d postinjury (Fig. 6), suggesting that a very small proportion of cells may migrate for short distances.

View larger version (102K): [in this window] [in a new window]   Figure 6. Time course of OEC tract formation and fill of lesion cavity. A–L, GFP (green) and GFAP (red) composite double-fluorescent immunolabeling over progressive times from lesion and cell grafting to death, demonstrating morphology of OEC tracts and filling of lesion cavity. Cell "tracts" extending from injection site (IS) to lesion site (Les) are present within 1 h of grafting. Over time, the lesion cavity fills, in part as a consequence of cell division (Fig. 9). By 3 d after injury, a cellular matrix of OECs is well established in the lesion site. Scale bars: (in K) A, C, E, G, I, K, 350 µm; (in L) B, D, F, H, J, L, 50 µm.

 
The OEC tract does not form when injected into other spinal cord locations or at low volumes
To further understand mechanisms underlying tract formation, OECs were transplanted in several different paradigms. These additional groups were killed 7 d after transplantation, a time point at which the groups described in the preceding section clearly exhibited cell distribution into tracts extending into the lesion site. When OECs were injected exclusively into gray matter located 1 mm rostral and 1 mm caudal to the lesion site immediately after injury, OECs remained in the injection site and did not form a tract between the injection and lesion site (Fig. 7). Thus, injection away from the gray/white matter interface and away from white matter tracts did not support formation of a tract into the lesion site. When a very low volume of cells was injected into the dorsal column white matter, 1 mm rostral and caudal to the lesion site immediately after injury, OECs remained primarily in the injection site and did not form a tract extending to the lesion site (Fig. 7). When OECs were injected into the dorsal columns at a distance 3 mm rostral and 3 mm caudal to the lesion site immediately after spinal cord injury, cells also remained in the injection site and did not form cell tracts (Fig. 7). When cells were injected into the dorsal column white matter in intact subjects, OECs remained primarily in the injection site (Fig. 7). These results indicate that the formation of a tract of OECs extending from the injection to the lesion site occurs only when cells are injected into white matter or at the gray/white interface, relatively close to the lesion site. Furthermore, OECs formed tracts to the lesion site only if grafted acutely after injury: among subjects that received injections of OECs into the dorsal columns either 3 d before injury or 9 d after injury, cells were detectable in the injection site but not in the lesion site (Fig. 7). When introduced 9 d after injury, some OECs aligned along the rostral–caudal orientation of white matter at the margins of the injection site, but migration was not evident and lesion cavities were devoid of cells (Fig. 7). At the site of one injection made 3 d before the C4 lesion, the caudal injection was located only 150 µm from the subsequent lesion cavity rather than the intended 1 mm; even in this case, the cavity was virtually devoid of OECs (Fig. 7).

View larger version (143K): [in this window] [in a new window]   Figure 7. OECs do not form tracts after injection at greater distances from lesion, or after injection of small volumes. A, OECs (green) do not form tracts extending to lesion cavity when injected into gray matter (GM) rather than white matter (WM), 1 mm rostral or caudal to the lesion site (Les). GFAP labeling (red) indicates lesion margins; the lesion cavity is empty (inset). IS, injection site. B, OECs do not form tracts extending to lesion cavity when small volumes (50 nl) are injected 1 mm rostral and 1 mm caudal (inset, arrowhead) to lesion site, at the same time that lesions are placed. C, OECs do not form tracts extending to lesion cavity when injected 3 mm rostral or caudal to the acute lesion site. D, OECs do not migrate when injected into the intact spinal cord. E, OECs injected 3 d before a lesion do not fill the lesion cavity. Cells within the caudal injection site (IS; right) are located 150 µm from the lesion cavity rather than the intended 1 mm distance; even with a large number of OECs in close proximity to the lesion, a distinct tract fails to form and only a rare cell is present in the otherwise empty lesion cavity. No cells appear adjacent to the lesion cavity in association with the rostral injection site (left), located 1 mm rostral to the lesion. F, OECs do not form tracts extending to the lesion cavity when injected 9 d after a lesion, 1 mm rostral or caudal to the lesion site. Scale bar: A, D, 175 µm; B, E, 350 µm; C, F, 630 µm.

 
Cell tracts also form after implantation of marrow stromal cells or fibroblasts
To address whether cell tract formation and filling of the lesion cavity is a unique characteristic of OECs after rostrocaudal transplantation, we transplanted GFP-expressing primary MSCs or fibroblasts 1 mm rostral and 1 mm caudal to an acute dorsal column lesion site. A time course study once again showed that cell tracts extending continuously from injection site to lesion cavity were present as early as 1 h postinjection after injection of either fibroblasts (Fig. 8A–F) or MSCs (Fig. 8G). Like OECs, both cell types filled the lesion cavity by 3–7 d. These results demonstrate that cell tract formation and filling of the lesion cavity can occur with other cell types, and are not unique to OECs.

View larger version (107K): [in this window] [in a new window]   Figure 8. Other cell types form tracts to the lesion site when injected acutely after injury. A–F, GFP and GFAP double-fluorescent immunolabeling indicates that fibroblasts also form tracts extending from the injection site (IS) to the lesion cavity (Les) when injected into dorsal white matter, 1 mm rostral or caudal to the lesion site. The time course of cellular distribution and filling of the lesion cavity entirely parallels that of OECs and MSCs (data not shown). G, Similar responses are observed after injection of bone marrow stromal cells (example of cells 3 h after injection is shown). Scale bars: A, C, E, G, 350 µm; B, D, F, 50 µm.

 
Cell proliferation contributes to lesion cavity filling
To test whether proliferation of transplanted cells contributes to cell filling of the lesion cavity, we performed intraperitoneal injections of BrdU (50 mg/kg/d) on each of the first 6 d after cell injection/injury. Double-confocal immunolabeling revealed that 20–40% of GFP-expressing OECs colocalized with BrdU in cell injection sites, cell tracts, and lesions (Fig. 9). These results indicate that OECs proliferate after in vivo injection, likely contributing to expansion of cell number over time.

View larger version (107K): [in this window] [in a new window]   Figure 9. OEC proliferation 1 week postgrafting. A, Triple-fluorescent immunolabeling for injected OECs (green; expressing GFP), BrdU (red) and astrocytes (GFAP; blue). OECs proliferate in the rostral–caudal injection sites (IS), cell tracts and lesion site (Les). B, Higher magnification of confocal Z-stacks from boxed area in A shows that many GFP-expressing OECs colocalize with BrdU. C, xy, xz, and yx plane images of typical GFP and BrdU double-labeled cells. Scale bars: A, 175 µm; B, 47 µm; C, 7 µm. D, Quantification demonstrates that 25% of GFP-labeled OECs have incorporated BrdU, 7 d postlesion (no significant groups differences at any site). Error bars indicate SEM.

 
Host Schwann cells penetrate OEC grafts and associate with regenerating axons
To examine the association of regenerating axons in OEC grafts with the local cellular milieu, we performed triple confocal high-resolution labeling for neurofilament, GFP (labeling implanted OECs), and the Schwann cell-specific marker 27C7 (Fig. 10) in grafts 1 month postimplantation. Most host axons present within grafts were associated with 27C7-labeled host Schwann cells, which migrated into the lesion/graft site, paralleling previous observations in fibroblast (Jones et al., 2003) and bone marrow stromal cell (Lu et al., 2005) grafts in SCI lesion sites. As noted above, host axons in the graft did not exhibit preferential topographical association with GFP-labeled OECs.

View larger version (98K): [in this window] [in a new window]   Figure 10. Schwann cells penetrate OEC grafts in lesion cavity and associate with penetrating axons. A, Composite image of graft in lesion site 1 month after injury, containing grafted OECs labeled for GFP (green), host Schwann cells labeled with the Schwann cell-specific marker 27C7 (red), and host axons labeled for NF (blue). B–E, The boxed region of A is shown at higher magnification. Host neurofilament-labeled axons penetrating the graft exhibit topographical association with Schwann cells (arrows). Scale bar: A, 16 µm; B–E, 6 µm.

 

	Discussion

Top Abstract Introduction Materials and Methods Results Discussion References

 
Findings of this study suggest that OECs exhibit neither unique migratory properties in relation to sites of spinal cord injury, nor enhanced axonal growth-promoting capabilities compared with other cellular substrates grafted into this lesion paradigm. In stead, we find that any of three cell types examined form continuous tracts extending into a spinal cord lesion site when injected 1 mm rostrally and caudally, and that the formation of these linear tracts is influenced by the timing, location, and volume of injection rather than cell type. Furthermore, we find that OECs do not support bridging of CST axons into or beyond a spinal cord lesion site. OECs did support, independent of tract formation, penetration of axons types other than the corticospinal system into a lesion cavity, but the degree of this axon growth did not differ from that of either fibroblast or bone marrow stromal cell grafts. OEC tracts displaced astrocyte processes, an effect that might reduce glial scars at lesion margins but could also alter blood–brain barrier repair after injury (Faulkner et al., 2004).

OECs have been described previously as cells that, in the adult, retain the ability to migrate toward the olfactory bulb after loss of axonal contact after olfactory nerve injury (Doucette, 1995). However, two recent studies indicate that OECs neither migrate nor proliferate in response to olfactory nerve injury, instead remaining as a conduit of cells that can guide regenerating axons of the olfactory nerve (Williams et al., 2004; Li et al., 2005). In this manner, they appear to function analogously to Schwann cells after a peripheral nerve injury. In addition, OECs actively phagocytose degenerating axons (Li et al., 2005). It has been proposed that the maintenance of open OEC channels plays a role in facilitating growth of axons from newly regenerated receptor neurons to their targets within the olfactory bulb (Li et al., 2005).

OECs have been reported to migrate extensively in the injured spinal cord, especially when transplanted rostrocaudally in proximity to a lesion site (Ramon-Cueto and Nieto-Sampedro, 1994; Li et al., 1998; Ramon-Cueto et al., 1998; Imaizumi et al., 2000a; Boruch et al., 2001; Keyvan-Fouladi et al., 2003; Resnick et al., 2003; Sasaki et al., 2004). It has been proposed that OECs might respond to signals or factors from injured neurons and their processes, therefore migrating preferentially toward an injury site (Ramon-Cueto et al., 1998; Boruch et al., 2001). However, based on our results, the formation of an OEC tract extending toward the lesion site from the site of grafting is most likely a pressure injection phenomenon caused by the rostrocaudal arrangement of glia and supporting tissue in spinal cord white matter. Indeed, there exists an extensive literature in the field of fluid flow dynamics in the brain and spinal cord describing the preferential movement of mass along the longitudinal orientation of white matter tracts (Rosenberg et al., 1980; Zhang et al., 1992; Bjelke et al., 1995; Geer and Grossman, 1997; Wood et al., 1999). The extensive movement of cells and fluid along these tracts is a function of the longitudinal orientation of cells, axons and their myelin sheaths within white matter (Zhang et al., 1992; Bjelke et al., 1995; Geer and Grossman, 1997). After a lesion, an injected substance would likely diffuse along this longitudinal axis and down a low-pressure gradient toward a lesion site. Previous studies have not examined other cell types as controls for OECs, and have not examined very early time points after cell injection, likely contributing to the potentially mistaken attribution of unique migratory properties to OECs.

Previous studies reported migration of OECs over extensive distances beyond a spinal cord lesion site based in part on the use of Hoechst cell labeling (Ramon-Cueto and Nieto-Sampedro, 1994; Ramon-Cueto et al., 1998, 2000; Boruch et al., 2001; Resnick et al., 2003; Cao et al., 2004; Chuah et al., 2004). However, subsequent reports indicated that the Hoechst label leaks from transplanted cells, leading to spread of the label rather than the implanted cell, causing an artifactual appearance of cell migration (Iwashita et al., 2000; Ruitenberg et al., 2002; Andrews and Stelzner, 2004). Consistent with our present results in a spinal cord injury paradigm, we previously xenotransplanted GFP-labeled lamina propria OECs into a dorsolateral funiculus crush lesion, and found very limited migration of OECs from injection sites (Ramer et al., 2004a; Richter et al., 2005). We now find in a syngenic grafting paradigm, characterized by excellent graft cell survival, that OECs rarely migrate beyond their site of injection.

Injection of OECs in this study did not support regeneration of corticospinal tract axons, and did not influence the growth of other axonal populations to extents differing from fibroblasts, bone marrow stromal cells or Schwann cells implanted into sites of injury in this and previous studies (Xu et al., 1995; Tuszynski et al., 1996; Liu et al., 1999; P. Lu et al., 2001, 2005). Furthermore, we observed no evidence that host axons used OEC tracts as "bridges" to enter or exit grafts, and tracts of OECs outside the lesion site were associated with an absence or reduction of axon density compared with the surrounding spinal cord. Instead, axons in the lesion site appear to preferentially associate with infiltrating Schwann cells after OECs have been transplanted into both focal and compressive SCI lesion models (Boyd et al., 2004; Ramer et al., 2004a). Such migration of endogenous Schwann cells is also observed after implantation of fibroblasts, bone marrow stromal cells, and stem cells into sites of SCI (Jones et al., 2003; Lu et al., 2005; Hill et al., 2006). Our findings contrast with previous reports that OECs promote bridging of axons into and beyond sites of SCI; it is possible that previous studies, which used either contusion or transection models, visualized spared rather than regenerating axons. For example, axons visualized as emerging from an OEC graft could instead be spared axons below a lesion that enter the graft from the caudal direction, rather than extending out of the graft and into the caudal spinal cord. Distinguishing whether an axon visualized below a lesion is extending rostrally or caudally is extremely complex in incomplete lesion models, particularly contusion models. We have directed considerable effort to assuring that the wire-knife lesions used in the present experiment completely transect corticospinal axons, by combining pressure applied downward with the upward movement of the wire knife against the dorsal columns and dorsal corticospinal tract (Weidner et al., 2001; Lu et al., 2004).

OECs normally support the extension of axons from newly born olfactory neurons in the olfactory bulb throughout life (Barnett, 2004). However, when olfactory axons are transected, these axons die back, the soma degenerates, and the axon does not regenerate (Graziadei and Monti Graziadei, 1980; Doucette et al., 1983; Doucette, 1990; Williams et al., 2004; Li et al., 2005). Hence, in the mature olfactory bulb, OECs do not stimulate axonal regeneration; rather, they support axonal extension from newly born neurons throughout life. Similarly, in the spinal cord, we find that OECs provide a cellular matrix in a lesion site; this matrix is penetrated by Schwann cells, and collectively this matrix supports host axonal growth to a degree paralleling that of other grafted cell types. We do not find a propensity of OECs to migrate or otherwise support directed axonal extension or corticospinal tract regeneration. Findings of the present spinal cord injury model yield no evidence that OECs stimulate axon growth more extensively than other cell types, and yield no evidence that OECs support axonal regeneration beyond a lesion site. The rationale for using these cells in extensive human experimentation now underway is therefore unclear. The rationale for use of these cells in chronic human injury is further limited by a recent report that these cells fail to support functional recovery in rodent models of chronic SCI (Steward et al., 2006).

	Footnotes

 
Received July 28, 2006; accepted Sept. 17, 2006.

This work was supported at the University of California at San Diego by National Institutes of Health Grant R01 NS09881, the Veterans Administration, the Canadian Spinal Research Organization, the Swiss Institute for Research into Paraplegia, and the Neuroscience Microscopy Shared Facility. This work was supported in Vancouver by the International Spinal Research Trust and the Christopher Reeve Paralysis Foundation.

Correspondence should be addressed to Mark H. Tuszynski, Department of Neuroscience, University of California at San Diego, La Jolla, CA 92093-0626. Email: mtuszynski{at}ucsd.edu

Copyright © 2006 Society for Neuroscience 0270-6474/06/2611120-11$15.00/0

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