The Journal
of Neuroscience,
December
1987, 7(12): 38273839
Cholinergic Innervation of the Smooth Muscle Cells in the Choroid
Coat of the Chick Eye and Its Development
Stephen
D. Meriney”
and
Guillermo
The University of Connecticut,
Pilar
Department of Physiology and Neurobiology, Storrs, Connecticut
The mechanical
and pharmacological
characteristics
of the
cholinergic
activation
of the smooth muscle in the choroidal
coat of the chick eye have been assessed
in tissues isolated
from birds 1 d posthatching
using histological,
electrophysiological,
and immunological
techniques.
The choroidal
coat
is innervated
by a dense network
of cholinergic
nerves that
make enpassantsynapses
with smooth muscle. Thirty-hertz
stimulation
of these nerves
initiates
red blood cell (RBC)
movement
in the vessels
of the choroidal
coat, and this
activation
is blocked
by muscarinic
ACh receptor
(AChR)
antagonists.
Force-transducer
recordings
of nerve-induced
contractions
of this tissue have a slow onset and relaxation
time course similar to those of smooth muscle contractions.
Furthermore,
since nearly half the cholinergic
neurons
innervating
the choroid die within a defined
period during development,
the onset and pharmacology
of this innervation
were studied
during
embryogenesis.
With a neural cytoskeletal-like
immunostain,
we demonstrated
that choroid axons are present
in peripheral
tissue by stage (St) 29. Extracellular
electrical
recordings
made
after
choroid
nerve
stimulation
allowed
us to distinguish
axon from muscle responses.
These procedures
permitted
us to examine
the
time course of the innervation
of the smooth
muscle. However, to visualize
the postsynaptic
smooth muscle response,
it was necessary
to treat the isolated preparation
with tetraethylammonium
chloride (TEA). Accordingly,
TEA-enhanced
electrical
smooth muscle
responses
to single-nerve
stimuli
could be recorded
only after St 39. Treatment
of the nervemuscle preparation
with prostigmine
allowed the recording
of TEA-enhanced
electrical
activity
as early as St 36 (1 d
after the beginning
of the normal choroid neuron death period). This synaptic
activation
was completely
blocked
by
atropine
or quinuclidinyl
benzylate
(QNB), and was not affected by alpha bungarotoxin
(aBTX), indicating
that, as in
the posthatching
tissue, neuromuscular
transmission
is mediated by muscarinic
receptors.
These results show that cho-
Received Jan. 27, 1987; revised June 8, 1987; accepted June 11, 1987.
We thank L. Landmesser. L. Dahm. and D. B. Grav for critical evaluation of
the manuscript, M. J. Spring for artwork, and S. Putnam for her editorial assistance.
This work was supported by NIH 10338, NSF-BNS 841058 1, and The University
of Connecticut Research Foundation.
Correspondence should be addressed to Dr. Guillermo Pilar, The University
of Connecticut, Department of Physiology and Neurobiology, 75 N. Eagle&
Rd., Rm. 416 U-42, Storm, CT 06268.
=Present address: Jerry Lewis Neuromuscular Research Center, UCLA School
of Medicine, 700 Westwood Plaza, Los Angeles, CA 90024.
Copyright 0 1987 Society for Neuroscience 0270-6474/87/123827-13$02.00/O
06266
linergic muscarinic
activation
of the choroidal
as early as St 36, but that it is not as efficient
later in embryogenesis.
coat can occur
as transmission
The choroidal coat of the vertebrate eye is essentially a vascular
rete that lies between the sclera and retina and encapsulates the
vitreous body. Early studies of the peripheral distribution of
efferent nerves from the parasympathetic chick ciliary ganglion
described the projection of some of these nerves to the choroid
coat (Marwitt et al., 1971) but a detailed study of this innervation has not been done. In this paper, a more complete description of the innervation and its development is presented.
The determination of the time of onset and the pharmacology
of transmission in this tissue during embryogenesis is important,
because nearly half the neurons from the cholinergic population,
which will eventually innervate this tissue, die during a defined
developmental time period. It has been shown that the neurons
in the ciliary population compete among themselves in the target
region (the iris and ciliary body) (Pilar et al., 1980), and it has
been assumed that the choroid population also engagesin competition for survival. Since it is known that the survival of these
neurons depends on the presence of the target (Landmesser and
Pilar, 1974), a detailed description of the development of the
cholinergic innervation of the choroidal coat is required for the
interpretation of observations of neuronal death following ACh
receptor (AChR) blockade (see Meriney et al., 1987).
There are other reasons that this study may be of general
interest. The retina of birds is avascular, and Rochon-Duvigneaud (1943) suggested that the choriocapillaris (a part of the
choroidal coat; see below) may be responsible for nourishing
the outer layers of the retina. In addition, since the pigmented
epithelial cells can transport ions at a rapid rate (Noel1 et al.,
1965; Lasansky and de Fisch, 1966) and appear to be responsible
for at least part of the transretinal potential, it is possible that
the choroid may serve as a source and sink of ions involved in
the epithelial transport processes. Furthermore, the pharmacological and contractile characteristics of the choroid are also
of clinical interest, since cholinergic activation of this tissue may
regulate blood flow and intraocular pressure.
In this work, we describe morphological characteristics of the
cholinergic muscarinic innervation of this tissue at the lightand electron-microscopic levels, and the pharmacology of the
choroid muscle’s contractile response to choroid nerve stimulation in the posthatching chick. We describe also the organization of the choroid coat. These observations are extended to
the study of the development of the cholinergic innervation of
the choroid coat during embryogenesis, with emphasis on the
3828
Meriney
and Pilar * Cholinergic
Innervation
of the Choroid
Deriod of normal cell death at stage (St) 34-40. We define the
time of the onset of innervation,
functional
neuromuscular
transmission,
and appearance
of AChRs on the postsynaptic
-
\
I
muscle cells of the choroid.
Materials
and Methods
White Leghorn chick embryos were incubated in a forced-draft incubator to the desired stage (Hamburger and Hamilton, 195 1). Choroid
tissue from chicks of embryonic and posthatch ages was dissected out
intact with the sclera, retina, and pigment layers. The same region of
the choroid was used for all experimental procedures. This region is
defined by an isosceles triangle whose apex is the point at which the
choroid nerves pierce the sclera, and whose base is the border of the
ciliary body. One side is bounded by the ciliary nerves, and the other
side is determined by the equal lengths of one side and the base, which
create the isosceles triangle. A superfusion solution ofTyrode’s was used
with 134 mM NaCI, 3 mM KCI, 20 mM NaHCO,, 3 mM CaCl,, 1 mM
MgCl,, and 12 mM glucose. Drugs were added to the superfusion solution
and their effects recorded at the indicated intervals. ACh, alpha bungarotoxin (orBTX), d-tubocurarine chloride (dTC), and atropine sulfate
were obtained from Sigma Chemical Co. (St. Louis, MO). Tetraethylammonium
chloride (TEA) was obtained from J. T. Baker Chemical Co. (Phillipsburg, NJ). Prostigmine and quinuclidinyl
benzylate
(QNB) (generously provided by Dr. P. Sorter) were obtained from Roche
(Nutley, NJ).
Electron microscopy. The tissue from 1-d-old chicks was fixed in 1.5%
glutaraldehyde,
1.5% paraformaldehyde,
and 1.5% acrolein in 0.1 M
cacodylate buffer (pH 7.3) for 5 hr. Specimens were postfixed in 2%
osmium tetroxide for 1 hr and dehydrated for embedding in Eponaraldite such that transverse thin sections could be cut on an ultramicrotome. Thick (1 pm) sections were mounted on glass slides and stained
with toluidine blue. Thin sections were mounted on #200 mesh grids
and sequentially stained with 2% uranyl acetate and 1.5% lead citrate
for viewing with a Phillips 300 electron microscope. Photograph montage reconstructions of large areas (200 pm2) of the choroid coat allowed
the identification of all cell types and their organization in this tissue.
Neural cytoskeletal-like immunostaining
of choroid axons. Wholemount preparations of choroidal tissue were separated from the sclera
and retina and pinned to the bottom of a Sylgard-coated 35 mm tissue
culture dish. The pigment layer adhered to the choroid in most young
embryos (St 34-40), and was removed by gently rubbing with a cotton
bud. These whole-mounts were dipped in dry-ice-cold acetone for 15
set, washed several times, and incubated overnight in phosphate-buffered saline with 0.3% Triton X-100 (PBST). A mouse hybridoma supematant (generously provided by H. Tanaka and L. Landmesser; see
Yamamoto et al., 1986), specifically directed against an as-yet undefined
neural cytoskeletal element, was incubated with the choroid tissue for
1 hr, followed by several changes in PBST and fixation with 4% paraformaldehyde. This antibody has been observed to stain the neurites of
chick spinal cord motoneurons from their earliest outgrowth throughout
development. This was determined by comparing its staining to that of
a second monoclonal directed against a motoneuron-specific
cell surface
antigen (L. Landmesser, unpublished observations). In addition, this
antibody stains neuritic outgrowth from cultured chick spinal motoneurons (L. Landmesser and L. Dahm, unpublished observations). The
cytoskeletal antigen was visualized under a fluorescent microscope after
incubation in goat anti-mouse tetramethylrhodamine
isothiocyanate
(TRITC) conjugate (1:50) for 45 min and mounting on glass slides;
photographs were taken for permanent records.
Observations of blood flow in the choroid coat. To determine the
response of the choroidal vessels at various embryonic ages to choroid
nerve stimulation and ACh application, the ciliary ganglion was surgically removed, together with the postganglionic choroid nerves and a
large piece of choroidal tissue, and placed in heparinized Tyrode’s. The
sclera, retina, and pigment were removed, and the choroidal coat was
pinned to the bottom of a Sylgard-coated perfusion chamber. Red blood
cells (RBCs) were observed in choroidal vessels under Hoffman-modulafion contrast optics (x 200) in this isolated tissue “sheet.” Following
either 30 Hz choroid nerve stimulation or pressure application of 50 ~1
drop 1 mM ACh solution, the number ofvessels in the &hole microscopic
field in which a movement of RBCs occurred was noted and scored.
India ink-Jill of choroid vasculature. To visualize the vascular bed in
the choroid coat, hatchling chicks were anesthetized with methoxyflurane and heparinized saline was injected into the ventricle of the heart,
followed by a 1 ml injection of Carter’s ink. Chicks were immediately
decapitated and chor&dal tissue was removed, isolated, mounted in
glycerine as described for immunostaining,
and observed with light
microscopy. Photographs were taken for permanent records.
Mechanical responses recorded from choroid muscle fibers. To determine the pharmacology and contractile characteristics of nerve-induced
choroid activation in the hatched chick, mechanical recordings of muscle tension were made in isolated choroid coat. Tension is generated in
this tissue by activation of smooth muscle cells and is measured with
a force-transducer. With these recordings, we are unable to determine
whether the mechanical response results from vasoconstriction, vasodilation of the blood vessels, or contraction of the suspensory ligaments
(see below). It is likely that the responses observed are a combination
of more than one of these elements and the result of the geometry of
the recording situation, which was manipulated to maximize the amplitude of the response. Since we are unable to determine from which
part of the organ the contraction originated, we have avoided ascribing
a functional role for the cholinergic activation, and only refer to a
movement of blood cells.
The effects of dTC, orBTX, and atropine on the synaptic activation
of the choroid muscle contractions were ascertained in preparations
where the ciliary ganglion was surgically removed with the choroid
nerves and a wedgelike piece of the choroid coat. The distal end of the
choroid (near the ciliary body insertion into the sclera) was lifted free
of the sclera on one side and of the retina on the other, and tied directly
to the homemade strain gauge. The choroid nerves were stimulated at
20 Hz at their emergence from the ciliary ganglion, and contractions in
the choroid coat were monitored on a chart recorder.
Surgical denervation of the choroid. To determine the contribution of
the ciliary ganglion to the innervation of the choroidal coat, a surgical
denervation was performed. Hatchling chicks were anesthetized with
methoxyflurane,
and a small incision was made between the eye and
the opening of the auditory canal to gain access to the posterior portions
of the optic cup. The eye was retracted and the ciliary ganglion was
located by blunt dissection. All postganglionic (ciliary and choroid)
nerves leaving the ganglion were cut with iridectomy scissors and, in
most cases, the ganglion was also completely removed. The success of
the surgery was evaluated 2, 3, or 4 d later, when the choroidal coat
was removed for immunohistochemistry.
We used only those birds that
had no pupillary response in the operated eye, no connection between
the ciliary ganglion and the sclera, and a vascularized choroidal coat
that appeared healthy.
Extracellular recording of TEA-enhanced electrical activity. For extracellular recording of electrical activity in the choroid, the ciliary
ganglion was dissected intact with the choroid nerves and a piece of the
choroidal coat. The sclera, pigment, and retinal layers were gently removed from the choroid to allow a recording suction electrode access
to the tissue. Suprathreshold single stimuli were delivered via a suction
electrode to the postganglionic choroid nerves, and electrical activity
recordings were stored via a digitizer (PCM- 1: Medical Svstem. Greenville, NT) and a Sony Beta HirFi Stereo Video Cassette kecorher (SLHF500). Prostigmine (10m6 gm/ml) and/or TEA (5 mM) were added to
the Tyrode’s solution superfusing the preparation, and activity was recorded at regular intervals, depending on the age ofthe chick. Embryonic
preparations were stimulated once per minute to reduce fatigue of embryonic synapses. The ability of atropine (2 FM), QNB (10 nM), and
olBTX (7.5 rglml) to modify the activity recorded in the choroid coat
was also evaluated.
Extracellular recording of isolated control choroid nerves was used
as a comparison for the responses to TEA and prostigmine recorded in
intact peripheral choroid tissue. To evaluate the frequency response of
activity recorded in either the choroid tissue or choroid nerves themselves, the tissues were stimulated at 20 Hz, and responses were continuously recorded for 15-25 sec. At regular intervals following the onset
of the repetitive stimulation, the square of the area under the extracellular waveform was measured on a digital oscilloscope (7854 Textronix;
Beavertown, OR) and plotted as a function of time.
Results
Cholinergic
innervation
of the mature organ
Choroid nerves leaving the ciliary ganglion pierce the sclera at
5-7 locations near the exit of the optic nerve and radiate over
the choroidal coat (Fig. 1). Major choroidal vessels diverge from
The Journal of Neuroscience, December 1987, 7(12) 3829
3830
Meriney
and Pilar
l
Cholmergic
Innervation
of the Choroid
India ink-fill ofthe choroidalvasculature.The densevascular
bed that permeatesthis tissueis clearly delineated.Calibration, 15 Wm.
Figure2.
the entrance into the sclera to create a dense vascular bed that
breaks up into a capillary network between arterioles and venules (see Fig. 2). Most of the choroidal volume is made of lacuriae, which consist of large endothelial-lined fluid reservoirs,
connected to the blood vessels. We have not determined whether
there are lacunae between capillaries or large vessels, but we
observed lacunae connected to arterioles by narrow openings
formed by endothelial cells wrapped by innervated smooth muscle cells. This heavily vascularized choroidal tissue forms a complete cuplike structure over the entire back of the eye, surrounding the vitreous humour.
Neuronal cytoskeletalimmunoreactivity and changesfollowing denervation.In the hatched chick, the density of innervation
was observed following indirect immunofluorescence staining
with a monoclonal antibody to an undefined neural cytoskeletal
element. Figure 3, A, B, demonstrates the dense network of
nerve fibers that runs between the large arterioles and venules
(V) but does not heavily innervate them. The densest innervation appears around small vessels (v) in the choroidal coat
(right, Fig. 3B).
Since both sympathetic and parasympathetic nerves innervate
the choroid, the parasympathetic ciliary ganglion was surgically
removed to determine the contribution of cholinergic nerves to
the innervation observed by immunostaining (Fig. 4A). Two
days after parasympathetic nerve denervation, the density of
staining decreased dramatically such that only a few nerves
remained (not shown). The possibility that a few sensory fibers
had been surgically cut cannot be excluded. However, the degree
to which sensory fibers innervate the choroid is unknown. This
low density of innervation persisted for 4 d after parasympathetic denervation (Fig. 4B), presumably owing to the presence of
a small number of sensory and/or sympathetic fibers. Kirby et
al. (1978) have described the presence of a scarce adrenergic
innervation of the choroid, which is in agreement with our
conclusion that the vast majority of the immunoreactive nerves
observed in the choroid coat clearly originate from the ciliary
ganglion.
Ultrastructural observationsof the innervationof the choroid.
The tissue organization of the choroidal coat can be seen in the
transverse 1 pm section shown in Figure 5. At the bottom of
this light photomicrograph are the outer layers of the retina (R).
The pigment epithelium layer can be seen running between the
photoreceptor cells of the retina and Bruch’s membrane (b). The
layer of the choroid coat closest to the retina is the choriocapillaris (c), which is followed by the larger vessel layers containing
RBCs (v). The walls of the large vessels have ridgelike outcroppings that sometimes connect adjacent vessels and presumably
serve some suspensory function, as suggested by Rochon-Duvigneaud (1943). The intravascular “suspensory” processesare
composed of smooth muscle cells embedded in a collagen matrix. Choroid nerve branches (n) filled with myelinated axons
usually run near the scleral edge of the choroid and subsequently
branch into muscle nerves. Muscle nerve branches are unmyelinated and many axon profiles contain dense accumulations
of small, clear vesicles (not shown). Within the choroidal coat,
terminal axon branches run in groups and are usually bound
together by Schwann cell processes that at least partially surround each fiber. At apparent “transmission” sites, vesicles fill
varicose axons (Fig. 6 A, B, V), which occasionally appose muscle membranes. There is no thickening or other apparent synaptic specialization of the nerve or muscle membranes. This en
passant type of innervation is often seen in smooth muscle
tissue, such as the vas deferens (Me&lees, 1968) and urinary
bladder (Tachibana et al., 1985).
There were 2 different stages represented among the differentiated smooth muscle cells in the choroid coat at hatching. A
layer of differentiated arteriole smooth muscle cells was easily
identified, it lay immediately adjacent to the endothelial wall
of the vessel and did not appear to receive innervation (not
shown). We assume that the activation of this muscle is mediated by blood-borne chemical factors. The smooth muscle
found in the outer layers of the arterial walls and in the suspensory ligaments was much less differentiated at hatching. Electron-microscopic montages of large areas of the choroid coat
were made to ease identification of cell types in this tissue.
Elongated smooth muscle cells were easily observed in these
montage reconstructions and allowed the characterization of the
partially undifferentiated smooth muscle cells, since most of the
contractile filaments were restricted to the elongated tips of the
cells (Fig. 6 A, l). In regions surrounding the cell nucleus, a
bulging of the cell was observed, and the cytoplasm contained
a very active Golgi apparatus (Fig. 6A, g) and endoplasmic
reticulum. As described above, these smooth muscle cells received a dense innervation. All of these features are displayed
from different cells in Figure 6A, as montage reconstruction of
an entire smooth muscle cell is cumbersome to present in a
figure.
Choroid musclepharmacologyand contractileresponses.
Since
The Journal of Neuroscience, December 1997, 7(12) 3831
Figure 3. Undefined neuronal cytoskeletalimmunoreactivity (seeMaterials and Methods) in the hatchling chick. Fluorescence(A) and phasecontrast(B) microaranhsof the samefield reveal that the densitv of innervation is highestaround smaller vessels(v), as largeones(V) are wrapped
by nerve‘bundles&ly. Calibration, 15 pm.
the cholinergic innervation of the choroidal coat is thought to
mediate vasodilation in the mammal, a change in blood flow
following parasympathetic nerve stimulation would be expected. Accordingly, 30 Hz choroid nerve stimulation conspicuously
moved blood in the vessels of the isolated choroid tissue (discussed in more detail below). Therefore, to measure the contractile response of smooth muscles that may be associated with
this blood movement, a sensitive force-transducer was used to
record contractions in the hatched chick. No responses to singlenerve stimuli were obtained, and noticeable contractions of the
choroid coat were present only after 3 or more stimuli (at 50
Hz) were delivered to the postganglionic choroid nerves (Fig.
74. Contractions of the choroid coat had a slow onset and time
course and were frequency-dependent (Fig. 7B), with an optimal
frequency of stimulation of between 30 and 50 Hz for maximal
force generation.
In the hatched chick, the choroid neuromuscular junction is
blocked by atropine (Fig. 84 c) and is not affected by dTC (Fig.
8A, b), or even by high doses (15 &ml) of aBTX (Fig. 8B, b).
In Figure 8, A, a and B, a, the control contractions elicited by
30 Hz stimulation applied to the choroid nerves are shown.
These results indicate that this junction is muscarinic. However,
the use of strain-gauge measurements of muscular contractions
to characterize this neuromuscular junction during development
is difficult. Our transducer was not sensitive enough to record
any force generated by embryonic choroid muscle. In addition,
developing nerve terminals would not be expected to be able to
follow the frequency stimulation required to generate force in
the choroid, since immature nerve terminals are known to fatigue very rapidly (see Fig. 11).
Development of cholinergic choroid innervation
TEA-enhanced electrical activity in embryonic choroid muscle.
To expose the embryonic choroid neuromuscular transmission,
we recorded extracellular electrical activity in the choroid tissue
following a single suprathreshold nerve stimulus. At all embryonic ages examined (St 35-hatching), extracellular action potentials were recorded with a 10 msec latency in almost all areas
of the choroid target tissue (Fig. 9A). Since this activity was not
affected by either muscarinic or nicotinic AChR antagonists, it
appears to have been due entirely to presynaptic nerve action
potentials. The inability to record postsynaptic muscle activity
extracellularly is not surprising, since smooth muscle often responds to nerve stimulation with subthreshold slow, graded
potentials that do not usually generate action potentials (Axelsson, 1970). These slow, graded potentials would not have
been recorded by our extracellular electrode.
To detect electrical activity in the choroid smooth muscle,
we attempted to induce action potentials in this normally “silent” tissue. Since TEA is known to block the rectifying K+
current in many tissues (Armstrong, 1966), it has been used to
depolarize and induce “spiking” in some smooth muscles
3832
Meriney
and Pilar - Cholinergic
Innervation
of the Choroid
Figure 4. Immunostain of nerve fibers in a 4-d-posthatch control chick choroid (A), and of nerve fibers denervated 4 d after surgical section of
all the choroid nerves (B). The dramatic decrease in staining indicates that most of the fibers observed with this antibody in A stain nerves emanating
from the ciliary ganglion. Calibration, 15 pm.
(R). Several
Figure 5. A 1 pm section of the choroid and surrounding tissue. The choroid is sandwiched between the sclera (5’) and the retina niocapillaris.
vessels filled with RBCs can be seen (v), as can a large choroid nerve bundle (n) between 2 lacunae (I). b, Bruch’s membrane, c, chc
Calibration, 20 pm.
The Journal
of Neuroscience,
December
1987, 7(12) 3833
Figure 6. Electron micrographsof presumptive cholinergic endingsin the choroid coat. Clear vesiclesfill varicose synaptic endings(v), which
occasionallycloselyapposesmooth muscle fibers (M). A, A group of varicoseaxonsruns betweenseveralsmooth musclefibers nearthe scleraledge
of the choroid (SW, scleralmatrix). Thesesmooth musclecells have a very active Golgi apparatus(g) nearnuclearregions,and contractile filaments
v) in distal tips of the cell. B, Higher magnification of a different region of the choroid where severalvaricoseaxons (V’),partially surroundedby
a Schwanncell (s), run near a smooth muscle cell (M). Calibration, 1 pm.
(Droogmans et al., 1977). Interestingly, TEA has a unique influence on smooth muscle: it blocks K+ channels following extracellular exposure (Holman and Neild, 1979), whereas it has
been shown to be effective in axons only when applied intracellularly (Armstrong, 1966). In the chick choroidal coat, superfusion with 5 mM TEA enhanced extracellularly recorded
electrical activity in response to nerve stimulation such that a
new, longer-latency compound action potential was recorded in
the choroid tissue (Fig. 9B, arrow). This effect occurred 3-5 min
after the onset of TEA superfusion and disappeared 3-5 min
later (Fig. 9C). This transient appearance of detectable activity
is presumably due to the time course of TEA-induced depolarization in the smooth muscle. As the membrane potential of
the smooth muscle approaches threshold, single-nerve-induced
postsynaptic depolarizations are enough to drive the muscle to
fire an action potential. However, this drive is presumably lost
as the TEA further depolarizes the tissue. Therefore, the TEAenhanced electrical activity was probably not a result of changes
in the activity of muscle nerves, and was most likely the result
of action potentials generated in postsynaptic muscle cells.
The pharmacology of the TEA-enhanced activity was investigated to determine if this muscle response was mediated via
muscarinic synaptic activation. At all ages, atropine (2 PM) or
QNB (10 nM) completely blocked the longer-latency TEA-enhanced activity without affecting the shorter-latency nerve activity (Fig. 10, A and C are controls, while Fig. 10, B and D are
3834
Meriney
and Pilar * Cholinergic
Innervation
of the Choroid
set
B
1
!
5mg
Figure 7. Choroid muscle contractions of the hatched chick in response to postganglionic choroid nerve electrical stimulation. A, Single (not
shown) or double pulses applied to the choroid nerves do not elicit a mechanical response (upper truce). A slow, protracted response is seen after
3 (middle traces) or 4 (lower truces) pulses. B, Choroid muscle contractions depend on frequency of stimulation. Upper trace, 10 Hz; middle trace,
33 Hz; lower trace, 50 Hz.
B
1:
C
I1 5w
Psec
Figure 8. A, Effect
contraction. b, dTC,
muscle after choroid
tetanic contraction.
of dTC and atropine on choroid muscle contractions elicited by postganglionic nerve stimulation (33 Hz). ~1,Control tetanic
1 PM, does not influence the tetanic contraction. c, Atropine, 1.5 PM, completely blocks the generation of force in the choroid
nerve stimulation. B, Effect of aBTX on choroid muscle contrations elicited by choroid nerve stimulation (33 Hz). a, Control
b, orBTX, 75 pgml, added to the superfusion solution does not influence the tetanic contraction.
The Journal
ii
I
0.1
mV
10 msec
Extracellular recording of electrical activity in the choroid
coat following single-shockstimulation of the choroid nerves (St 44).
A, Control. B, TEA, 5 mM, enhancesmuscular activity such that it can
be recordedextracellularly. C, Wash. In this figure and in Figures 10,
12, and 13, the arrow indicates the TEA-elicited response.
Figure 9.
responses after TEA application). In addition, aBTX (7.5 wg/
ml) was unable to affect the nerve- or TEA-enhanced activity
(Fig. 10, arrow) (Fig. lOE, control; Fig. lOF, after TEA). These
results indicate that the TEA-enhanced activity is synaptic, and
of Neuroscience,
December
1987, 7(12) 3835
that this choroid neuromuscular synapse is muscarinic throughout embryonic development. Pretreatment of the preparation
with prostigmine increased the amplitude of the synaptic TEAenhanced electrical activity-further
proof that this activity is
cholinergic (discussed below).
Since TEA may be influencing axons as well as muscle electrical activity, extracellularly recorded compound action potentials from isolated choroid nerves were monitored after perfusion with TEA (not shown). After 6 min of TEA perfusion, no
changes in the size and only small changes in the shape of nerve
action potentials were noticed. If the TEA perfusion was continued for 30 min, however, a broadening of the nerve action
potential became apparent. This long-term effect of TEA on
choroid nerve action potentials is not likely to have contributed
to the enhanced activity recorded in the intact choroid tissue,
since the long-latency muscle electrical activity recorded always
appears 3-5 min after the onset of TEA perfusion and, in fact,
disappears.
The frequency response of both nerve- and TEA-enhanced
activity to 20 Hz nerve stimulation was examined between St
42 and hatching (Fig. 11). The responses from both isolated
choroid nerves (Fig. 11, open circles) and muscle nerves (closed
circles) recorded within peripheral choroid tissue decreased
slowly and at a similar rate. In contrast, TEA-enhanced activity
decreased very rapidly (2 set) during 20 Hz nerve stimulation
(see Fig. 11, triangles). This is a further indication that this
electrical activity is postsynaptic, since embryonic synaptic
transmission is known to fail during high-frequency stimulation.
This failure of synaptic transmission is similar to that seen in
embryonic iris junctions (Pilar et al., 198 1) and developing frog
neuromuscular junctions (Letinsky, 1974).
To determine the effective onset of transmission in this tissue
(sufficient to activate a postsynaptic response), the effects ofTEA
on extracellular potentials recorded in the choroid were examined between St 35 and hatching. In Figure 12, it can be seen
that TEA has no effect on eliciting a response at St 36; Figure
12A is the control response, Figure 12B is after TEA application,
and Figure 12C is 10 min after TEA. The earliest developmental
stage at which TEA was able to enhance electrical activity (arrow) was St 39 (Fig. 12, D-F’). To determine whether the de-
C
E ;
-\rr
Ik..i
10
msec
Figure IO. Pharmacology of the TEA-enhanced activity. All recordings from St 40. A, Control. B, Atropine, 2 PM, added to the superfusate
completely blocks a responseto 5 mM TEA. In another preparation (C), 10 nM QNB also completely blocks the responseto 5 mM TEA (D).
However, the electrical responseto TEA is not blocked by the nicotinic AChR blocker (uBTX. E, Control. F, aBTX, 7.5 pg/ml, + TEA, 5 mM.
3838
Meriney
and Pilar * Cholinergic
Innervation
of the Choroid
10 msec
P-
0
i
i
lb
1'5
i
J/p-
-lo.’
mV
i0
TIME (WC)
Figure II.
Frequency response of nerve (solid lines) and TEA-enhanced (dashed line) extracellularly recorded electrical activity (St 42).
Choroid nerve stimulation (20 Hz) begins to slowly fatigue the compound action potential recorded in isolated choroid nerves (0) after 5
sec. The activity recorded extracellularly in muscle nerves ofthechoroid
coat (0) shows an early decline, probably due to terminal axon branch
block at this high frequency, but the fatigue levels off to parallel that
observed in isolated choroid nerves. The TEA-enhanced activity recorded in the choroid coat (A) fatigues very rapidly during a 20 Hz
choroid nerve stimulation. Vertical lines, mean + SEM.
velopmental
appearance
of this TEA enhancement (St 39) was
at the earliest embryonic age at which nerve stimulation could
induce
muscle
activity,
cholinergic
transmission
recordings
made
in the absence
F
i
I----
iI
was facilitated
by prior superfusion with prostigmine. TEA was able to enhance
the electrical activity in prostigmine-treated tissues as early as
St 36 (Fig. 13, A-C) and increased the size of TEA responses
after St 39 (Fig. 13, D-F), which provides evidence for some
transmission as early as St 36. These records were compared to
previous
c4 i i
Jl
of prostigmine
10
(not
msec
Figure 13. Prostigmine enhancement of TEA-enhanced electrical activity. A 30 min superfusion of prostigmine (lo6 gm/ml) allows the
recording of a TEA-enhanced response as early as St 36 (A-C). A, Control after prostigmine. B, TEA, 5 mM, enhances activity such that a
small response is observed after the nerve action potential. C, Wash.
In addition, prostigmine enlarges the response at older embryonic ages
(D-F, St 39). D, Control after prostigmine. E, TEA, 5 mM, produces a
large muscle response. F, Wash.
which served as controls. This enhancement
of the TEA
electrical activity by prostigmine is further proof that these responses are cholinergic and postsynaptic. The prostigmine treatment required at these early embryonic ages may be necessary
because the amount of ACh released from terminal varicosities
shown),
might
mitter
Figure 12. The developmental appearance of TEA-enhanced electrical
activity. At St 36 (A-C), there is no response ta TEA. A, Control. B,
TEA, 5 mM. C, Wash. The earliest developmental stage at which TEA
enhances extracellularly recorded electrical activity is St 39 (D-F). D,
Control. E, TEA, 5 mtvr. F, Wash.
not yet be sufficient, or the distance over which the transmust diffuse is longer than it is later in development
(see
first paragraph of Discussion in Meriney et al., 1987).
Developmental appearance of cytoskeletal immunoreactivity.
Developing choroid nerves reached the peripheral target area
long before we were able to record choroid neuromuscular transmission (St 36). By St 29, neural cytoskeletal immunoreactivity
demonstrated the growth of choroid axons into the periphery
(Fig. 14A). By St 33, these axons began to ramify and traverse
most of the choroidal coat (Fig. 14B). However, a dense network
of nerves did not begin to form until St 38 (Fig. 14C). As the
chick matured, the network of nerves became very thick, and
densely covered the choroidal tissue (Fig. 140). These observations indicate that choroidal nerves are present in the periphery before the onset of transmission, and gradually ramify
to densely innervate the choroidal muscle, presumably at the
time that electrical recordings of the TEA-enhanced response
are possible.
Observations of bloodjlowfollowing ACh or nerve stimulation.
To determine when the choroid could respond to ACh appli-
The Journal of Neuroscience, December 1987, 7(Q)
Developmental appearanceof choroid nerves (observedby immunostaining) in the choroid coat. A, At St 29, choroid nervesare
spreadingover the peripheral tissue.B, By St 33, the nervesbegin to ramify and traversemost of the peripheralarea. C, By St 38, a network of
fibers beginsto innervate the choroid. D, At St 43, an increaseddensity of innervation is observed.All micrographsare from the same identified
region of the choroid (seeMaterials and Methods).
Figure 14.
cation or nerve stimulation with a contraction sufficient to move
blood in the choroidal vessels, RBC movement was observed
at various developmental time periods (see Table 1). Thirtyhertz stimulation of the choroid nerve was required to move
blood cells in choroidal vessels, but it could do so only after St
44. This is not surprising, since embryonic nerve terminals would
be expected to fatigue with repetitive stimulation (see Fig. 1 I).
ACh application, however, was able to induce RBC movement
as early as St 36. Both nerve- and ACh-induced blood flow was
blocked by atropine, indicating that the response is muscarinic
and begins at about the same time as does the TEA-prostigmineenhanced electrical activity in the choroid coat. It is possible,
however, that the ACh-induced blood flow at early embryonic
ages is primarily due to activation of the more differentiated,
and most likely uninnervated, inner layer of arteriole smooth
muscle. Therefore, although this indicates that AChRs are present, we cannot determine whether this activation is relevant to
cholinergic innervation, since we have not observed innervation
of these early-differentiating arteriole smooth muscle cells.
Nevertheless, we can conclude that functional AChRs appear
3838
Meriney
and Pilar * Cholinergic
Table 1. Observations
stimulation
Embryonic
day
8
Innervation
of blood flow following
nerve or ACh
Response to
Embryonic
stage
ACh
-
34
36
38
40
42
44
10
12
14
16
18
of the Choroid
3 dph
+
+
+
++
+++
30 Hz
+
+++
+++
If blood flowed in most of the vessels observed, + + + was scored. If about half
responded, + + was scored, and if only several responded, + was scored. When
no blood flow was observed following chemical or electrical stimulation, - was
scored.
on contractile
muscle by St 36. It is also possible that AChRs
are present on precursors of smooth muscle cells that we cannot
detect with our method.
Discussion
The vascular choroid coat lining the back of the eye has been
described in the monkey and rabbit (Ruskell,
196 1, 1970; Bill,
1962), but the cholinergic
innervation
of this structure in mammals is not well understood.
In mammals,
the source of parasympathetic
innervation
arises from the sphenopalatine
ganglion and mediates
vasodilation
(Ruskell,
197 1). Adrenergic
nerves also innervate
choroid blood vessels, and sympathetic
activation
results in vasoconstriction
(Bill, 1962). In the present
work, we describe the parasympathetic
cholinergic
innervation
of the choroid in the chicken by the ciliary ganglion. We have
shown that the choroid cholinergic
motoneurons
of the ganglion
project into the choroid coat and ramify by about St 33, but
they do not initiate
muscular
activity in the smooth muscles
until St 36. In vitro, measurement
of this early muscular
activation requires the presence of the anticholinesterase
(prostigmine). In addition,
we have shown that choroid neuromuscular
synapses are entirely muscarinic from embryonic stages to
hatching.
The regulation of blood flow in the choroid is particularly
important in birds, since there is no central artery of the retina.
The functions of this innervation in birds revolve around alterations in blood flow in this heavily vascularized tissue. When
the postganglionic choroid nerves leaving the ciliary ganglion
are repetitively stimulated, RBCs move in the vessels of the
choroid. It is possible that this regulation of blood flow involves
a parasympathetic retinal reflex pathway, described by Reiner
et al. (1983).
Since the choroid
may provide
the major
blood
supply to the outer layers of the retina, metabolic demands
resulting from retinal illumination may be met by increased
blood flow through the choriocapillaris. The choriocapillaris
may also be involved in the regulation of ionic transport across
the pigment epithelium. It is of interest that an increase in blood
flow within the mammalian eye has been demonstrated following an increase in retinal illumination (Parver et al., 1982). The
choroid may also play a role by preventing damage of the retina
by increasing blood flow during changes in ambient light levels.
Photoreceptors
in the retina
have
been shown
to degenerate
following blockage of choroidal blood flow (Gay et al., 1964;
Golder
and Gay,
1967) or sustained
exposure
to slightly
higher
than normal levels ofillumination (Lanum, 1978). Furthermore,
intraocular pressure would be very sensitive to changes in choroidal blood flow. It is possible that the lacunae serve as a liquid
reservoir and regulate intraocular pressure by filtering fluid out
of the blood vessels. The choroid coat innervation previously
described may be important in regulating intraocular pressure.
Glaucoma, one of the leading causes of blindness in mammals,
occurs when intraocular pressure is high enough to causedamage
to nerve fibers in the retina. This disorder is normally treated
with anticholinesterases, which presumably produce vasodilation and decrease intraocular pressure. An understanding of the
regulation of intraocular pressure and its control by the innervation described in this work may be useful as a model for
studies of intraocular pressure changes in mammals.
The characterization of the innervation of the choroid may
be critical to the processes described above, but it is also important embryologically, since the number of cholinergic motoneurons innervating the choroid is reduced by about 50%
during a critical time in development. Neuromuscular interactions between motoneurons and skeletal muscle have been
studied extensively; however, these observations have not previously been extended to the motor innervation of smooth muscle. The ciliary ganglion-choroid smooth muscle system is well
suited to these studies because of the compact and peripheral
location of the motoneurons and the accessibility of the choroid
smooth muscle. These data are essential to the experimental
study described in the following paper (Meriney et al., 1987)
on the normal neuronal death among the choroid motoneurons.
It is interesting that, as in other tissues, choroid motor nerve
processesare present in the target environment before the onset
of the normal neuronal death. However, unlike the well-studied
skeletal neuromuscular junction, they do not make functional
synaptic contacts until St 36 (at least 1 d after the onset of the
cell death). This implies that competitive interactions between
choroid motoneurons and choroidal targets may exist before
functionally effective transmission begins, an idea discussedmore
fully in the subsequent paper (Meriney et al., 1987).
References
Armstrong, C. M. (1966) Time course of TEA-induced anomalous
rectification in squid giant axon. J. Gen. Physiol. 50: 491-503.
Axelsson, J. (1970) Mechanical properties of smooth muscle, and the
relationship between mechanical and electrical activity. In Smooth
Muscle, E. Bulbring, A. F. Brading, A. W. Jones, and T.Tomita, eds.,
DD. 298-314.
Williams & Wilkins. Baltimore. MD.
Bill: A. (1962) Autonomic nervous control of’uveal blood flow. Acta
Physiol. Stand. 56: 70-81.
Droogmans, G., L. Raeymaekers, and R. Casteels (1977) Electra- and
nharmacomechanical
counlina in the smooth muscle cells ofthe rabbit
ear artery. J. Gen. Physiol. 76: 129-148.
Gav. A. J.. H. Golder. and M. Smith (1964) Chorioretinal vascular
occlusions with latex spheres. Invest, ‘Ophthalmol. 3: 647-656.
Golder, H., and A. J. Gay (1967) Chorioretinal vascular occlusions
with latex microspheres (a long term study). Part II. Invest. Ophthalmol. 6: 5 l-58.
Hamburger, V., and H. L. Hamilton
(195 1) A series of normal stages
in the development of the chick embryo. J. Morphol. 88: 49-92.
Holman, M. E., and T. 0. Neild (1979) Smooth muscle: Membrane
properties. Br. Med. Bull. 35: 235-241.
Kirby, M. L., I. M. Diab, and T. G. Mattio (1978) Development of
adrenergic innervation of the iris and fluorescent ganglion cells in the
choroid of the chick eye. Anat. Rec. 191: 3 1 l-320.
Landmesser, L., and G. Pilar (1974) Synaptic transmission and cell
death during normal ganglionic development. J. Physiol. (Lond.) 241:
737-749.
Lanum, J. (1978) The damaging effects of light on the retina. Empirical
The Journal
findings, theoretical and practical implications.
Surv. Ophthalmol.
22: 221-248.
Lasansky, A., and F. W. de Fisch (1966) Potential, current, and ionic
fluxes across the isolated retinal pigment epithelium and choroid. J.
Gen. Physiol. 49: 913-924.
Letinsky, M. S. (1974) Physiological properties of developing frog
tadpole nerve-muscle junctions during repetitive stimulation. Dev.
Biol. 40: 154-161.
Marwitt, R., G. Pilar, and J. N. Weakly (1971) Characterization
of
two cell populations in the avian ciliary ganglion. Brain Res. 25: 3 17334.
Meriney, S. D., G. Pilar, M. Ogawa, and R. Nuiiez (1987) Differential
neuronal survival in the avian ciliary ganglion after chronic acetylcholine receptor blockade. J. Neurosci. 7: 3840-3849.
Menillees, N. C. R. (1968) The nervous environment of individual
smooth muscle cells of the guinea pig vas deferens. J. Cell Biol. 37:
794-817.
Noell, W. K., D. Crapper, and C. V. Paganelli (1965) Transretinal
currents and ion fluxes. In Transcellular Membrane Potentials and
Ion Fluxes, F. M. Snell and W. K. Noell, eds., D. 92. Gordon and
Breach, New York.
Parver, L. M., C. Auker, D. 0. Carpenter, and T. Doyle (1982) Choroidal blood flow. II. Reflexive control in the monkey. Arch. Ophthalmol. 100: 1327-1330.
of Neuroscience.
December
1987,
7(12) 3939
Pilar, G., L. Landmesser, and L. Burstein (1980) Competition
for
survival among developing ciliary ganglion cells. J. Neurophysiol. 43:
233-254.
Pilar, G., J. Tuttle, and K. Vaca (198 1) Functional maturation of motor
nerve terminals in the avian iris: Ultrastructure,
transmitter metabolism and synaptic reliability. J. Physiol. (Lond.) 321: 175-193.
Reiner, A., H. J. Karten, P. D. R. Gamlin, and J. T. Erichsen (1983)
Parasympathetic ocular control. Trends Neurosci. 6: l-6.
Rochon-Duvigneaud,
A. (1943) Les yeux et la vision des vertebres,
p. 452, Masson, Paris.
Ruskell, G. L. (1961) Aqueous drainage paths in the rabbit. Arch.
Opthalmol. 66: 86 l-864.
Ruskell, G. L. (1970) An ocular parasympathetic
nerve pathway of
facial nerve origin and its influence on intraocular pressure. Exp. Eye
Res. 10: 319-330.
Ruskell, G. L. (197 1) Facial parasympathetic innervation of the choroidal blood-vessels in monkeys. Exp. Eye Res. 12: 166-172.
Tachibana, S., M. Takeuchi, and T. Fugiwara (1985) Visualization of
autonomic varicose terminal axons by scanning electron microscopy.
J. Electron Microsc. 34: 136-138.
Yamamoto,
M., A. M. Boyer, J. E. Crandall, M. Edwards, and H.
Tanaka (1986) Distribution of stage-specific net&e-associated
proteins in the developing murine nervous system recognized by a monoclonal antibody. J. Neurosci. 6: 3576-3594.