EXPERIMENTAL NEUROLOGY
ARTICLE NO.
143, 45–60 (1997)
EN966318
Fetal Spinal Cord Transplants Rescue Some Axotomized Rubrospinal
Neurons from Retrograde Cell Death in Adult Rats
FUTOSHI MORI,*,† B. TIMOTHY HIMES,*,‡ MASAYOSHI KOWADA,† MARION MURRAY,*
AND
ALAN TESSLER*,‡
*Department of Neurobiology and Anatomy, The Medical College of Pennsylvania/Hahnemann University,
Philadelphia, Pennsylvania 19129; †Department of Neurosurgery, Akita University School of Medicine,
1-1-1 Hondo, Akita City, Akita 010, Japan; and ‡The Philadelphia Veterans Administration Medical Center,
Philadelphia, Pennsylvania 19104
the site of a complete spinal cord transection (45) or,
after a delay, into an incomplete contusion injury (67).
The mechanisms by which transplants enhance locomotor performance are unknown.
Rescue of neurons from axotomy-induced retrograde
cell death represents one possible mechanism. Fetal
spinal cord transplants keep alive all the 35–40% of the
ipsilateral Clarke’s nucleus neurons at the L1 segment
that would otherwise die after hemisection of the
midthoracic spinal cord of either newborn or adult rats
(27). They also prevent death of all the 56% of the
contralateral red nucleus (RN) neurons that die after
midthoracic spinal cord hemisection in newborn rats
(12). Rubrospinal neurons atrophy (20, 68, 72) and die
(20, 22, 50, 60, 72) after axotomy in adults, but it has
not yet been determined whether transplants rescue
RN neurons in these animals. One aim of the present
investigation was to provide this information.
In both newborns and adults, transplants are thought
to rescue axotomized neurons at least in part by serving
as a surrogate source of target-derived neurotrophic
factors (12, 18, 24, 27). Additional mechanisms may
apply, however, and these are likely to differ in newborns and adults. After spinal cord injury in newborns,
for example, interrupted and late-developing supraspinal axons are able to grow through transplants and into
caudal host spinal cord, where they appear to establish
connections with their normal targets (4, 8). This has
provided part of the evidence suggesting that growth
and synapse formation favor permanent survival of
axotomized neurons (9, 12, 38). Growth into intraspinal
fetal spinal cord transplants has also been observed in
adult recipients, but this is largely restricted to axons
whose perikarya are located within 0.5 mm of the
transplants; only rare supraspinal axons grow into
these transplants in adults (32). A second goal of the
present study was to examine whether the spinal
projections of RN neurons that survive axotomy can
extend into fetal spinal cord transplants and into
caudal host spinal cord. Because the RN plays an
important role in the control of limb movement (42;
Intraspinal transplants of fetal spinal cord may contribute to recovery after spinal cord injury by keeping
axotomized neurons alive. In this study we examined
whether transplants rescued axotomized red nucleus
(RN) neurons from retrograde cell death in adult rats.
RN neurons were labeled by retrograde transport of
Fluorogold (FG); 1 week later right-sided RN neurons
were axotomized by left-sided hemisection at C3–4
vertebral level, and Embryonic Day 14 spinal cord or
gelfoam was introduced into the cavity. Additional rats
received hemisection and a transplant of fetal spinal
cord or gelfoam without FG injection. At 2 and 4
months, the number of neurons in the magnocellular
portion of the RN contralateral to the hemisection
decreased 35–40% in rats that received gelfoam; mean
soma area of surviving neurons decreased 40%. RN cell
loss was reduced to 20% in rats that received fetal
spinal cord transplants, but the decrease in mean soma
area was unchanged. Transplants therefore rescued
about half of the axotomized RN neurons that otherwise would have died but did not prevent perikaryal
atrophy. Anterograde transport of WGA–HRP injected
into RN 2 months after transplantation showed that
rubrospinal axons reached the site of injury but rarely
entered transplants; FG injections caudal to transplants showed that axons of transplant neurons extended at least two segments into host spinal cord.
Fetal spinal cord transplants may therefore contribute
to locomotor recovery in adults with spinal cord injuries both by preventing retrograde cell death and by
establishing novel circuits across the site of injury. r 1997
Academic Press
INTRODUCTION
Intraspinal transplants of fetal spinal cord enhance
the development of locomotor performance after the
spinal cord of newborn animals has been either completely transected (29, 31, 45) or overhemisected (11,
35). More limited recovery has been observed in adult
recipients when transplants were placed acutely into
45
0014-4886/97 $25.00
Copyright r 1997 by Academic Press
All rights of reproduction in any form reserved.
46
MORI ET AL.
reviewed in 28), we also examined the projections
formed between fetal spinal cord transplants and caudal host spinal cord. Information about the anatomical
connections between RN neurons and transplants and
between transplants and host spinal cord would provide additional insight into the mechanisms by which
transplants contribute to the recovery of locomotor
performance after spinal cord injury in adults.
MATERIALS AND METHODS
Animals
Sixty adult female Sprague–Dawley rats weighing
225–300 g (Zivic-Miller Laboratories, Allison Park, PA)
were used in these studies. Fourteen rats underwent
spinal cord hemisection alone, and 30 rats received
fetal spinal cord transplants into the hemisection site.
Eight age-matched animals served as intact, unoperated controls and 4 received fluorescent tracer Fluorogold (FG; Fluorochrome, Inc., Englewood, CO) injection
only as control. The surgical procedures were carried
out in accordance with the Laboratory Animal Welfare
Act Guide for the Care and Use of Laboratory Animals
(NIH, DHEW Publication No. 78-23, Revised 1978)
after review and approval by the Animal Care and Use
Committee of the Medical College of Pennsylvania/
Hahnemann University.
Spinal Cord Hemisection and Transplantation
After rats were deeply anesthetized with an intraperitoneal injection of xylazine (5 mg/kg), ketamine (50
mg/kg), and acepromazine (0.4 mg/kg), the spinal cord
was exposed by a partial laminectomy of the C3 and C4
vertebrae, and a hemisection cavity 3–4 mm in length
was formed in the left side of the spinal cord with
microscissors and gentle aspiration. The lesion completely severed the axons of the rubrospinal tract in the
ipsilateral lateral funiculus as well as the ipsilateral
dorsal and ventral funiculi and gray matter. In the
hemisection only group, the cavity was filled with
gelfoam soaked with saline. In transplant recipients,
the cavity was filled with one or two whole pieces of
Embryonic Day 14 (E14) spinal cord removed from
embryos of timed pregnant Sprague–Dawley rats. The
day of insemination was considered E0. The dura matter
was closed with interrupted 10-O sutures and covered with
a piece of hydrocephalus shunt film (Durafilm; Codman
Surlef, Inc.), the muscle and skin were closed in layers. The
techniques for transplantation have been more fully described in previous publications (12, 53).
Prelabeling of RN Neurons by Retrograde Transport
of Fluorogold
To determine that cells surviving hemisection in the
presence of transplants include RN neurons that had
been axotomized, we prelabeled neurons using the FG.
This procedure produces labeling of neurons that lasts
at least 2 months (27, 39) but does not cause degeneration of retrogradely labeled cells at concentrations
equal to or less than 2.5% (62). After the rats had been
anesthetized as described above and the spinal cord
exposed by C6 laminectomy, a single pressure injection
of 2% FG (2 µl) was made into both sides of the spinal
cord through a glass pipette (tip diameter 50–60 µm)
attached to a 10-µl Hamilton syringe. The wound was
closed as described above. One week later, the rats
underwent left-sided hemisection of the C3–4 spinal
cord with insertion of a spinal cord transplant or
gelfoam into the lesion cavity.
Tissue Processing and Staining
Animals survived 2 or 4 months after surgery. There
were no consistent differences in the results between
these survival times. For perfusion the rats received an
overdose of sodium pentobarbital (75 mg/kg, ip) and
were perfused through the left ventricle with phosphatebuffered saline (PBS) followed by fixative containing
4% paraformaldehyde and 0.02% picric acid in 0.1 M
phosphate buffer, pH 7.3. The perfused rats were then
positioned on a stereotaxic frame, the brain was divided into two parts in the plane of 7.0 mm from
bregma (48) and the brain stem and spinal cord were
removed. The tissue was cryoprotected by immersion in
an ascending series of 10–30% sucrose dissolved in 0.1
M phosphate buffer. In FG-injected rats, tissue blocks
containing the RN were serially sectioned at 16 µm on a
cryostat and every third section was mounted onto
gelatin-coated slides for analysis of FG-labeled neurons. The sections were air dried and briefly immersed
in xylene, coverslipped using DPX mounting media
(Fluka Chemical Co., Ronkonkoma, NY) and observed
with a fluorescence microscope. Additional 16-µm sections from both FG-injected and non-FG-injected rats
were directly mounted onto gelatin-coated slides for
Nissl–Myelin stain (15) or immunocytochemistry
(MAP1B, ED-1, OX-42, GFAP). The C3–4 spinal cord
was serially sectioned at 20 µm and stained with
Nissl–Myelin stain to confirm the completeness of the
hemisection and the presence of a transplant. Animals
were eliminated from the study if the hemisection did
not sever the ipsilateral lateral funiculus and gray
matter (N 5 2) or if no transplant remained in rats that
had received a transplant or if prominent cysts were
present at the rostral interface between host spinal
cord and transplant (N 5 4).
Cell Counting and Cell Size Analysis of RN
Neurons were counted in the magnocellular portion
of the RN at the level of the interpeduncular nucleus,
which comprises the caudalmost 480 µm of the RN (48,
TRANSPLANTS SAVE AXOTOMIZED ADULT RUBROSPINAL NEURONS
plate 24) and is the source of most rubrospinal axons
(13, 30, 52, reviewed in 58). In rats that did not receive
FG injections, the quantitative analysis was performed
on every third section stained for Nissl–Myelin; in rats
that received FG, the quantitative analysis was performed on every third section prepared for FG visualization as described above. RN neurons with a visible
nucleus were counted and the cell soma area was
measured with the Bioquant image analysis system
attached to a Leitz Dialux microscope at a final magnification of 3676 under bright-field illumination for
Nissl–Myelin stain and 3961 under fluorescent illumination for FG. Neurons were classified on the basis of
soma area as small (,300 µm2 ), medium (300–500
µm2 ), large (500–1000 µm2 ), or giant (.1000 µm2 ).
Corrected cell counts were obtained with the following
procedures. Nuclear diameters were measured at a
magnification of 31303 for 105 nuclear profiles from
both lesioned and unlesioned RN. These data were then
processed by means of the Hendry (26) analysis as
modified by Smolen et al. (66) to obtain a factor for
corrected neuron counts. Total neuron number was
determined by the formula (correction factor 3 raw cell
counts 3 distance between sections)/section thickness.
Because this correction factor assumes that the neuron
nucleus is a sphere, the present analysis provided
absolute numbers of neurons biased to the extent that
the shape of the neuronal nucleus differs from this
assumption (47). Stereological counting methods might
therefore provide different absolute numbers of neurons. Our primary interest was in side-to-side comparisons between right and left RN neuron numbers,
however, and these will be reliably determined by our
methods unless axotomy or transplantation changes
the extent to which the neuron nucleus can be considered to be spherical. Nuclear shape did not differ on
right and left sides. A paired t test was used to analyze
the numerical data for side-to-side differences within
groups for two variables: mean cell size and corrected
total cell numbers. The groups compared were normal
animals, animals with hemisection alone, and hemisected animals with a transplant of fetal spinal cord. In
all cases, analysis of the numerical data with a one-way
ANOVA showed that the RN of unoperated controls did
not differ statistically from the ipsilateral RN of lesioned animals in any group for any of the variables
measured. Therefore, we used the lesion/control ratio of
each animal as the basis for comparison. Overall significance of the ratio data was determined by the KruskalWallis one-way ANOVA (P , 0.05). If significance differences were present, individual post hoc comparisons
were made with the Mann–Whitney U test. All analyses were performed using the StatView statistical
computer program (Abacus Concepts, Berkeley, CA).
47
Immunocytochemistry
Antibodies raised against several cell-specific markers were used to ensure that cells counted in the RN
were in fact neurons, particularly because of the need
to distinguish neurons labeled with FG from macrophages and microglia that can phagocytose neurons
(56). These antibodies were (1) antimicrotubule-associated protein 1B (MAP1B), one of the components of
crossbridges between microtubules (61), which recognizes neurons; (2) ED-1, which recognizes an uncharacterized cytoplasmic antigen found in all cells of the rat
macrophage/monocyte line (17); (3) OX-42, which recognizes the complement C3bi receptor expressed by neutrophils, monocytes, macrophages, and microglia (59,
57); and (4) antiglial fibrillary acidic protein (GFAP),
which recognizes the major protein found in glial
intermediate filaments (5, 19), present in astrocytes
(36). The immunocytochemical methods were modifications of the procedures of Milligan et al. (43, 44). The
antibodies and dilutions used were (1) MAP1B (a
generous gift from Dr. Itzhak Fischer), a polyclonal
antibody diluted 1:250 (27, 59); (2) ED-1 (Harlan Bioproducts for Science, Indianapolis, IN), a monoclonal
antibody diluted 1:150 (27, 43, 44); (3) OX-42 (Harlan
Bioproducts for Science), a monoclonal antibody diluted
1:500 (28, 44, 45); and (4) GFAP (Biomedical Technologies, Inc., Stoughton, MA), a polyclonal antibody diluted 1:1000 (27). MAP1B was diluted in 0.1 M PBS, pH
7.4, containing 1% nonfat milk; the others in 0.1 M
PBS, pH 7.4, containing 4% nonfat milk. Sections were
incubated at room temperature overnight in a humid
chamber. After several rinses in PBS, the appropriate
peroxidase-conjugated secondary antibody was applied, also diluted in PBS containing nonfat milk: for
MAP1B and GFAP, a goat anti-rabbit IgG (Jackson
Immunoresearch Labs, Inc., West Grove, PA.) diluted
1:75; for ED-1 and OX-42, a goat anti-mouse IgG
(Jackson Immunoresearch Labs, Inc.) diluted 1:50.
Specific staining was visualized by incubating the
tissue with 3,38-diaminobenzidine tetrahydrochloride
(DAB; Sigma Chemical Co., St. Louis, MO) in distilled
water. The sections were then air dried, dehydrated,
and coverslipped with DPX mounting media and observed using bright-field microscopy.
Axon Tracing Studies
Two or 4 months after transplantation, retrograde
transport of FG was used to study the projections from
transplant neurons into caudal host spinal cord, and
anterograde transport of wheat germ agglutininconjugated horseradish peroxidase (WGA–HRP) was
used to identify projections between RN neurons and
transplants.
FG injection. Rats used for this study (N 5 6) were
not prelabeled by FG injections prior to transplanta-
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MORI ET AL.
FIG. 1. Nissl–Myelin-stained cross sections show (A) that the lesion completely severed the lateral funiculus, where the axons of the
rubrospinal tract course, and (B) that the transplants (TP) were well integrated with host spinal cord (H). Bar, 500 µm.
tion. They were anesthetized as described above and
their spinal cord exposed by laminectomy two segments
caudal to the transplants. A 2% FG solution (1 µl) was
pressure injected into the host spinal cord bilaterally as
described above. The dura was closed with interrupted
10-O sutures and covered with Durafilm, and muscle
and skin were closed in layers. Three days later the rats
were perfused as described. A spinal cord block containing the transplants and two segments of the adjacent
rostral and two segments of the adjacent caudal spinal
49
TRANSPLANTS SAVE AXOTOMIZED ADULT RUBROSPINAL NEURONS
cord including the injection site were removed and
immersed in an ascending series of 10–30% sucrose
dissolved in 0.1 M phosphate buffer. Frozen tissues
were cut at 20 µm on a cryostat. Every third section was
collected in consecutive order; additional sections were
stained for Nissl–Myelin. Sections for FG study were
processed as described above.
WGA–HRP injection. Two or 3 months after transplantation, the rats (N 5 8) were positioned on a stereotaxic apparatus and a burr hole made by a dental drill
according to the coordinates from a rat brain atlas (48).
The coordinates for the injection were 5.9 mm caudal
from the bregma, 0.7 mm from the midline, and 7.0 mm
from the dura matter of the brain. A 1% WGA–HRP
solution (Sigma Chemical Co.; 0.03–0.1 µl) was pressure injected into the right magnocellular RN neurons
through a micropipette (tip diameter 30–40 µm) attached to a 1-µl Hamilton syringe. Seventy-two hours
later the rats were anesthetized with an overdose of
sodium pentobarbital and perfused with 150 ml heparinized saline followed by 500 ml of fixative (1.25%
glutaraldehyde and 1% paraformaldehyde in 0.1 M
phosphate buffer, pH 7.4). Brain stem and spinal cord
segments were removed and immersed in an ascending
series of 10–30% sucrose in 0.1 M phosphate buffer. The
brain stem, including the RN, was cut coronally at 30
µm; the spinal cord was cut sagittally at 30 µm.
Midbrain and spinal cord sections were reacted immediately according to the tetramethylbenzidine procedure
described by (41) and counterstained with 1% neutral
red.
RESULTS
Spinal Cord Hemisection
The spinal cord lesion severed the left lateral funiculus at the C3–4 segments (Fig. 1A). Because rubrospinal tract axons are almost entirely crossed at this level
(reviewed in 58), the lesion axotomized neurons of the
RN on the right side of the midbrain and spared the left
RN. In all animals included in the quantitative study
(N 5 12), the lesion was limited to the left side of the
spinal cord and completely severed the dorsal, lateral,
and ventral funiculi and destroyed the gray matter on
the left side.
Transplant Morphology
Twenty-six of 30 recipients contained surviving transplants, and prominent cysts had not formed at the
rostral interface between host spinal cord and transplant. Transplants contained many mature neurons
and a neuropil that included both myelinated and
unmyelinated axons and resembled other intraspinal
embryonic spinal cord transplants that have been
described (12, 27, 53). The extent of gliosis at the
transplant–spinal cord interface varied among animals, but we included all animals in our quantitative
analyses and axon tracing studies except those with
cysts (Fig. 1B).
Effects of Axotomy and Transplants on RN Neuron
Survival and Size (Table 1)
In unoperated control rats the magnocellular portion
of the right and left RN contained similar numbers of
neurons, which were almost equally distributed into
small, medium and large classes; about 2% of cells were
giants (Figs. 2A, 3A). Neuron numbers in the left RN of
normal did not differ from those in the left RN of
operated rats 2 or 4 months after C3–4 left-sided
hemisection alone or hemisection plus transplant. Neuron cell size distribution and the mean soma area of left
RN in normals were also similar to those of experimental animals (Figs. 3B, 3C).
Two and 4 months after hemisection alone (N 5 8),
the number of neurons in the magnocellular portion of
the axotomized RN had decreased by 38% (Figs. 2B,
4B). The cell size distribution was markedly skewed
TABLE 1
Mean Cell Size and Cell Number in RN (Nissl–Myelin)
Mean cell size (µm2)
Group
Left
Right
Total cell number
Ratio (R/L)
Left
Right
Ratio (R/L)
Control, mean 6 SD (N 5 8) 463.830 6 39.920 465.070 6 47.278 1.003 6 0.059 1296.847 6 187.519 1287.358 6 183.881 0.997 6 0.089
Hemisection, mean 6 SD
(N 5 8)
462.213 6 22.096 291.236 6 16.195* 0.630 6 0.018 1340.331 6 152.103 833.650* 6 108.425 0.621 6 0.025
Transplant, mean 6 SD
(N 5 8)
433.201 6 34.609 283.992 6 25.576* 0.657 6 0.045 1327.518 6 185.824 1042.386 6 150.884* 0.785 6 0.032
Significant differences among groups**
Control . Hemisection, Transplant
Control . Transplant . Hemisection
* Right differs from left (P , 0.05) using paired comparison t test.
** Overall significant difference among group ratios was determined by Kruskal–Wallis one-way ANOVA (P , 0.05). Individual post hoc
comparisons made with the Mann–Whitney test.
50
MORI ET AL.
FIG. 2. Transverse section of RN about 400 µm rostral to the caudal pole. (A) Normal. (B) Left-sided hemisection. (C) Left-sided
hemisection with transplant. Note cell loss after hemisection (B) and partial preservation of cells in the presence of a transplant. Nissl–Myelin
stain. Bar, 200 µm.
TRANSPLANTS SAVE AXOTOMIZED ADULT RUBROSPINAL NEURONS
51
toward the small cell size, and giant cells were completely absent (Fig. 3B). The mean soma area of surviving neurons was 37% smaller than that of neurons in
the right RN (Fig. 4A).
In animals with hemisection and transplant (N 5 8),
about 80% of the normal number of neurons remained
in the magnocellular portion of the axotomized RN
(Figs. 2C, 4B). Transplants therefore rescued about half
of the RN neurons that would have died without a
transplant. As in the axotomized RN after hemisection
FIG. 4. Bar graphs representing mean 6 SD of (A) cell size and
(B) cell survival in RN as represented by the ratio of the neurons on
the lesion side (R)/neurons on the control side (L). (A) Mean cell size
decreased similarly in RN contralateral to the hemisection and to the
transplant. (B) 38% of cells died contralateral to the hemisection, but
only 20% died in the presence of the transplant. *, ,Nor. (normal); **,
,Tp. ,Nor. Data obtained from Nissl–Myelin-stained material.
alone, however, the neuron size distribution was shifted
toward the small cell size; the number of small neurons
increased to twice that of normal, and giant cells were
absent. The mean cell soma area was reduced to an
extent (35%) similar to that in the axotomized RN
following hemisection alone (Fig. 4A).
Survival of Rubrospinal Neurons (Table 2)
FIG. 3. Soma size distribution in RN in (A) normal, (B) after
left-sided hemisection, and (C) after left-sided hemisection plus
transplant. Cell size distribution is symmetrical in normal animals
(A). The distribution was markedly skewed to the small cell size after
hemisection (B) or after hemisection plus transplant (C). The change
in size distribution was similar in the two experimental groups.
Nissl–Myelin stain.
We first examined the number and sizes of magnocellular RN neurons projecting to the spinal cord by
injecting FG into the C6 spinal cord of normal rats
(N 5 4). Two months after injection, 66% of RN neurons
were FG labeled. There were no differences in cell
numbers or mean cell size between the right and left
RN. The mean size of FG-labeled neurons was 491 µm2.
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MORI ET AL.
TABLE 2
Mean Cell Size and Cell Number in RN (Fluorogold)
Mean cell size (µm2)
Group
Left
Right
Total cell number
Ratio (R/L)
Left
Right
Ratio (R/L)
Control, mean 6 SD (N 5 4) 493.562 6 20.434 487.687 6 11.585 0.989 6 0.040 804.562 6 99.690 825.562 6 94.191
1.032 6 0.103
Hemisection, mean 6 SD
(N 5 4)
504.930 6 33.786 344.592 6 34.484* 0.683 6 0.060 769.735 6 75.736 500.800 6 108.425* 0.654 6 0.043
Transplant, mean 6 SD
(N 5 4)
483.967 6 25.681 327.333 6 28.297* 0.676 6 0.041 795.973 6 26.859 669.223 6 47.219* 0.836 6 0.033
Significant differences among groups**
Control . Hemisection, Transplant
Control . Transplant . Hemisection
* Right differs from left (P , 0.05) using paired comparison t test.
** Overall significant difference among group ratios was determined by Kruskal–Wallis one-way ANOVA (P , 0.05). Individual post hoc
comparisons made with the Mann–Whitney test.
This was 10% larger than the mean cell size determined from adjacent sections stained for Nissl–Myelin.
Small neurons represent about 29% of neurons in the
magnocellular portion of RN; 35% of these were FG
labeled. Medium-sized neurons constitute 37% of the
neurons in the normal magnocellular RN; 84% were
labeled by FG. The large cells are 31% of the normal
neuron population; 94% were FG labeled. Giant cells
make up ,3% of the normal neurons; 65% were FG
labeled (Figs. 5A, 6A). Magnocellular RN neurons of all
sizes therefore send axons to the spinal cord, but even
some of the largest neurons do not.
Labeling magnocellular RN neurons with FG prior to
cervical hemisection and transplant enabled us to
compare the number of neurons projecting to the spinal
cord that survived axotomy with and without a transplant (28). Control RN of experimental animals had
neuron numbers and neuron size distributions similar
to those of unoperated animals. Two months after
hemisection alone (N 5 4), the axotomized RN contained 65% of the number of FG-labeled neurons present in the control RN (Fig. 5B). The mean size of
surviving axotomized FG-labeled neurons was 345
µm2; this was 32% smaller than in the control RN (Fig.
6B). Following transplantation of fetal spinal cord into
the hemisection cavity (N 5 4), the magnocellular portion of the control RN had neuron numbers and neuron
size distributions similar to those of unoperated control
animals. The magnocellular portion of the axotomized
RN contained about 84% of the neurons present in the
control RN (Fig. 5C). The mean size of labeled neurons
in the axotomized RN was 327 µm2; this was 32%
smaller than that in the control RN (Fig. 6C). These
results indicate that transplants rescue about half of
the magnocellular RN neurons projecting to the spinal
cord that were otherwise destined to die after axotomy,
but that transplants do not prevent atrophy of these
cells.
Immunocytochemistry
To confirm that the cells which we counted were
neurons (27), we stained sections of the RN with four
immunocytochemical markers that are specific for different cell types. Rats that survived for 2 months after
cervical hemisection (N 5 4) or hemisection plus transplant (N 5 4) were studied.
MAP1B (Fig. 7B). MAP1B was seen in the cell
bodies of larger RN neurons of normal animals. The
axotomized RN had fewer immunopositive cells in both
the hemisection alone group and the hemisection plus
transplant group. Cells in RN which were FG positive
were also MAP1B positive, identifying them as neurons.
ED-1. ED-1-positive cells were present next to blood
vessels (43, 44). The FG-positive cells were ED-1 negative, indicating that they were not macrophages or
monocytes.
OX-42. OX-42-positive cells were present in the
axotomized and control RN in both hemisection alone
and hemisection plus transplant groups. The FGpositive cells were, however, OX-42 negative, indicating that they were not microglia.
GFAP. GFAP was localized to the cell bodies and
processes of astrocytes in both axotomized and control
RN of all animals. FG-positive cells within the RN were
GFAP negative, indicating they were not astrocytes.
The results of these FG and immunocytochemical
studies therefore support the identification of the cells
we counted in the RN as neurons.
Axon Tracing Studies
Projections from transplant neurons into caudal host
spinal cord. In preliminary experiments FG injected
into segments adjacent to the transplant labeled large
numbers of host and transplant cells. To rule out
TRANSPLANTS SAVE AXOTOMIZED ADULT RUBROSPINAL NEURONS
53
FIG. 5. Fluorescence photographs of FG labeling (A) in normal RN, (B) after hemisection, and (C) after hemisection plus transplant about
400 µm rostral to the caudal pole. Note decreased number of labeled cells contralateral to the hemisection but sparing of cells contralateral to
the transplant. Bar, 200 µm.
spurious labeling through diffusion, further studies
utilized FG injections into host spinal cord two segments caudal to the transplant. These injections labeled by retrograde transport the perikarya of many
host neurons adjacent to the injection site. Fewer
labeled neurons were present in the transplants, and
the interface between host gray matter and transplants
was apparent because of a sharp decrease in the
number of labeled neurons between host spinal cord
and transplants (Figs. 8A, 8B). All of the transplants
that we studied (N 5 6) contained small numbers of
retrogradely labeled cells, which in some transplants
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MORI ET AL.
spread into surrounding white matter were not further
studied even if the RN was well labeled. In all of the
rats that received WGA–HRP and in which reaction
product was adequately seen (N 5 7/8), labeled axons
and collaterals with varicosities descended in the lateral funiculus of the host spinal cord contralateral to
the site of WGA–HRP application. Some of these axons
penetrated into the glial scar formed between the host
spinal cord and the transplant but did not extend into
the transplant or caudal host spinal cord (Fig. 10).
DISCUSSION
The results of these experiments show that cervical
hemisection of the adult rat spinal cord causes about
40% of the neurons present in the magnocellular portion of the contralateral RN to die and many of the
surviving neurons to atrophy; transplants of fetal spinal cord acutely placed into the hemisection site rescue
about half of these neurons from retrograde cell death
but do not prevent atrophy of the survivors; in the
presence of a transplant, axotomized rubrospinal axons
reach the level of the transplant, and, if rescued RN
neurons establish connections with neurons in the
caudal host spinal cord, these must occur via relays
across the transplants.
Axotomy Induces RN Neuron Death
FIG. 6. Soma size distribution of FG-labeled neurons in RN. (A)
In normal animals, all size classes of RN neurons project to cervical
cord. In (B) hemisected alone and (C) hemisected plus transplants
RN, the distribution was markedly shifted to the smaller sizes. The
results from FG labeling show the same pattern of atrophy as the
results from Nissl–Myelin preparations (Fig. 3).
formed clusters of labeled neurons. These were distributed throughout the transplants and were not preferentially located in the caudal regions closest to the site of
labeling. In no case were labeled cells observed rostral
to a transplant.
Projections from RN neurons to transplant. Injection of WGA–HRP into the rostral half of the right side
of the midbrain formed an injection site 500–700 µm in
length, which was largely centered on the magnocellular portion of the RN (Fig. 9). Cases in which the tracer
The present study has demonstrated a ,40% loss of
neurons in the magnocellular portion of the contralateral RN following hemisection of the cervical spinal
cord of adult rats. These counts, as well as those
showing transplant-mediated rescue, were obtained
from Nissl-stained material and confirmed by counts of
RN neurons labeled by retrograde transport of FG prior
to spinal cord injury. Counts of FG-labeled neurons
showed ,35% cell loss after cervical hemisection. The
cell loss determined by these two methods cannot be
directly compared since FG was applied at the C6
vertebral level, between two and three segments caudal
to the site of the spinal cord hemisection. Some axotomized neurons therefore were unlabeled by FG because
they terminated rostral to the site at which label was
applied (14, 65). We also cannot be certain about the
proportion of axotomized RN neurons that die; neurons
in the magnocellular portion of the RN that send axons
to spinal cord segments rostral to C3–4 escaped injury,
as did RN neurons that project elsewhere (reviewed in
58). Our immunocytochemical studies established that
FG-containing cells surviving in the RN were neurons
by showing them to be immunoreactive for MAP1B, a
neuron-specific marker (61), but not for ED-1, OX-42, or
GFAP, which identify macrophages, monocytes, microglia, and astrocytes.
Our conclusion that a portion of axotomized RN
TRANSPLANTS SAVE AXOTOMIZED ADULT RUBROSPINAL NEURONS
55
FIG. 7. Double staining of sections labeled with (A) FG and (B) an antibody to MAP1B to identify cells in RN contralateral to a hemisection
with transplant. (A) FG-labeled cells (arrows) are (B) MAP1B positive (arrows). A is a fluorescence photomicrograph. B is a brightfield
photomicrograph. The DAB reaction product obscures cytoplasmic FG labeling of MAP1B-positive neurons, but FG labeling remains visible
within the nuclei. Bar, 200 µm.
neurons dies agrees with several previous reports of
axotomy-induced retrograde cell loss in the RN after
spinal cord injury both in neonates (12, 50) and in
adults (20, 22, 60, 72). We cannot, however, exclude the
possibility that our cell counts overestimate the extent
of neuron death if some surviving neurons have atrophied below our level of detectability (68, 69) and do not
produce detectable levels of MAP1B. The cell loss that
we observed after hemisection of the cervical cord
exceeds that observed in adult rats after hemisection of
the thoracic cord (22, 50). This would be consistent with
greater vulnerability to axotomy close to the perikaryon (2, 21, 51), but is also due to axotomy of greater
numbers of RN neurons at the cervical than at the
thoracic level (69). Since RN neurons are also lost when
the spinal cord is compressed severely rather than cut
(71), these studies emphasize that neuron death is one
factor likely to limit recovery after both penetrating
and nonpenetrating spinal cord injury.
Our results do not allow us to distinguish whether
cells from all size categories of RN neurons were lost or
only a subset. We observed a 37% decrease in the mean
56
MORI ET AL.
FIG. 8. (A) Fluorescence micrograph showing retrogradely labeled neurons within the host spinal cord (H) and transplant (TP).
Arrowheads indicate host–transplant interface. FG was injected into
host spinal cord two segments caudal to the transplant. Bar, 200 µm.
(B) Four of the FG-labeled neurons in the transplant are shown at
higher magnification. Bar, 300 µm. (A) and (B) are from sagittal
sections.
cell size of RN neurons that survived axotomy for 2 to 4
months, but this shift could reflect a selective loss of
large and giant neurons, atrophy of these neurons or
both. Previous reports have demonstrated atrophy of
RN neurons after axotomy in both neonates and adults
(12, 50, 69, 72).
Transplants Rescue Some Axotomized Neurons
Transplants of embryonic spinal cord kept alive
about half of the axotomized RN neurons that would
have died in the absence of a transplant. Survival
appears to have been permanent; neurons were maintained for at least 2–4 months, the longest survival
periods studied, and their numbers did not decrease
further between 2 and 4 months. The mechanisms that
account for permanent rescue from axotomy-induced
retrograde cell loss, however, remain unknown. One
possibility is that transplants serve as a surrogate
source of neurotrophic factors that normally derive
from the targets of the rescued neurons and can be
taken up by the cut axons. Neurotrophic factors administered exogenously have prevented the death of immature axotomized motoneurons (63, 64, 73) and of several different types of axotomized neurons in adult
brain (1, 23, 25, 33, 34, 46, 69). Consistent with this
idea is the finding that transplants of embryonic CNS
tissues that are normal targets of RN neurons ensured
long-term survival of virtually all rubrospinal neurons
injured in newborn rats, but CNS tissues that are not
normal targets or sciatic nerve grafts produced only
temporary rescue (9, 12).
The available evidence indicates that brain-derived
neurotrophic factor (BDNF) and/or neurotrophin-3
(NT-3) are among the neurotrophic factors that may be
responsible for the transplant-mediated rescue of axotomized RN neurons. These are members of a family of
neurotrophins whose structure closely resembles that
of nerve growth factor (NGF) and which act on neurons
primarily through specific protein tyrosine kinase (trk)
receptors located on the cell surface (reviewed in 3).
NGF binds with greatest affinity to trkA, BDNF to
trkB, and NT-3 to trkC (reviewed in 3). RN neurons
express mRNA for trkB (40, 69, 70, reviewed in 3) and
trkC (69, 70), but not trkA (40, 69, 70; reviewed in 3),
suggesting responsiveness to BDNF and NT-3, but not
NGF. E14 spinal cord, the age of our transplants,
expresses high levels of mRNA for NT-3 and considerably lower levels of mRNA for NGF and BDNF (37).
Neither the presence nor the time course of expression
of the mRNA for neurotrophic factors nor the factors
themselves have been examined in transplants of embryonic spinal cord. The notion that transplantmediated rescue of axotomized RN neurons depends at
least in part on BDNF, however, receives support from
the finding that administration by gelfoam pledget at
the site of spinal cord hemisection in newborn rats
produces partial, but permanent rescue of axotomized
RN neurons from retrograde cell death (16). The superiority of transplants in rescuing axotomized RN neurons
in newborns suggests that transplants provide a single
neurotrophic factor in larger amounts or for a longer
time than does a gelfoam pledget or that survival
depends on multiple factors or additional conditions
which are satisfied by a transplant.
The contrast between transplant-mediated survival
of rubrospinal neurons that is virtually complete in
newborns and only partial in adults, despite the generally greater vulnerability of newborn neurons to
axotomy, is part of the evidence suggesting that transplants in some cases also contribute to permanent
TRANSPLANTS SAVE AXOTOMIZED ADULT RUBROSPINAL NEURONS
57
FIG. 9. Injection site of WGA–HRP into the rostral half of the right side of the midbrain which was largely centered on the magnocellular
portion of the RN (arrowheads). No labeled neurons are seen in the contralateral RN. Bar, 200 µm.
survival of injured neurons by providing a matrix that
allows continued axon growth and synapse formation
with target neurons (9, 12, 38). In the newborn rat,
regenerating or late-developing axons of corticospinal
and bulbospinal neurons, including rubrospinal, serotonergic, and other brain-stem neurons, grow through
fetal CNS transplants and into host spinal cord many
segments caudal to the transplant (6, 8, 10). In the
adult host spinal cord, however, most of the cell bodies
of neurons that send axons into transplants are located
within a few millimeters of the transplants, and even
these axons have not been shown to grow through the
transplants and into caudal spinal cord (32). In the
present investigation anterograde transport of WGA–
HRP showed many axons of surviving RN neurons
reaching as far as the glial scar at the transplant
interface, rare axons penetrating the transplant, and
none extending into caudal host spinal cord. This
contrasts with the results found with peripheral nerve
grafts placed into the cervical cord, which elicited or
supported regeneration by a few rubrospinal neurons
(55, 69). The explanation for this difference between
embryonic spinal cord transplants and peripheral nerve
grafts is unknown but is likely to be due to different
molecular environments. Failure to regenerate and
establish synaptic connections with target neurons in
caudal spinal cord may nevertheless contribute to the
inability of transplants to produce long-term survival of
all axotomized RN neurons in adults.
Transplants of embryonic spinal cord, cerebellum,
and neocortex secured the permanent survival of virtually all of the 35–40% of Clarke’s nucleus neurons at the
L1 segment that normally die after hemisection of the
adult or newborn spinal cord at T8 (27). The requirements for transplant-mediated cell rescue appear to
differ not only for newborn and adult neurons in RN,
but also among different populations of neurons in RN
and Clarke’s nucleus. The features of the neurons that
account for these differences remain to be identified.
The present investigation found that transplants did
not prevent perikaryal atrophy of adult RN neurons
that survived axotomy. Transplants also did not prevent atrophy of Clarke’s nucleus neurons that survived
ipsilateral hemisection of the spinal cord in adult or
newborn rats (27). In contrast, BDNF applied adjacent
to the RN has been reported to prevent perikaryal
atrophy of RN neurons after axotomy in adult rats (69,
70), and transplants of embryonic spinal cord into the
site of spinal cord hemisection prevent shrinkage of
surviving RN neurons in newborns (12). Neuron survival may therefore require smaller quantities of neurotrophic factors than are required to maintain perikaryal size. In the absence of continued growth and
contact with target neurons, as observed with severed
rubrospinal axons and transplants in newborns, transplants may fail to prevent or reverse perikaryal atrophy because they provide insufficient quantities of
neurotrophic factors to replace those supplied from the
normal targets.
Transplant Neurons Send Projections into Host
Spinal Cord
The results of the present investigation showed that
injection of FG two segments caudal to the transplants
labeled donor neurons by retrograde transport. Labeled
58
MORI ET AL.
efferent axons presumably entered host spinal cord by
penetrating regions of the host–graft interface where
they were not impeded by a glial scar. Outgrowth by
donor axons into host spinal cord has been reported
previously (32, 53). Our tracing studies of surviving
rubrospinal axons with anterograde labeling of RN
neurons revealed only an occasional labeled axon within
the transplants and none caudal to the transplants, but
many labeled axons terminated in host spinal cord just
rostral to the transplants. It is therefore possible that
neuronal relays were formed across regions of damaged
spinal cord via local axonal connections between host
spinal cord and transplants. Further studies will be
necessary to test whether such novel circuits were
established and their functional significance.
Intraspinal embryonic spinal cord transplants have
been shown to promote limited locomotor recovery after
several types of spinal cord injury in adults (45; reviewed in 7, 54). The present study has demonstrated
that partial rescue of axotomized supraspinal neurons
is one mechanism that may contribute to this recovery;
the establishment of functional relays across transplants represents a second possible mechanism.
ACKNOWLEDGMENTS
We are grateful to Brian Tryon for his contributions and to Theresa
Connors, Kathleen Bozek, Michael Spector, and Jean-Manuel Nothias for their technical assistance. The study was supported by NIH
Grant NS 24707 and the VA Medical Research Service.
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