Effects of 6-hydroxydopamine on primary cultures of substantia
nigra: specific damage to dopamine neurons and the impact of glial
cell line-derived neurotrophic factor
Yun Min Ding,1 Juliann D. Jaumotte, Armando P. Signore and Michael J. Zigmond
Department of Neurology and the Pittsburgh Institute for Neurodegenerative Disease, University of Pittsburgh School of Medicine,
Pittsburgh, Pennsylvania, USA
Abstract
6-Hydroxydopamine (6-OHDA)-induced loss of dopamine
(DA) neurons has served to produce an animal model of DA
neuron loss in Parkinson’s disease. We report here the use of
6-OHDA to produce an in vitro model of this phenomena using
dissociated cultures prepared from neonatal rat mesenceph-
alon. Cultures were exposed to 6-OHDA (40–100 lM, 15 min)
in an antioxidant medium, and DA and GABA neurons eval-
uated by immunocytochemistry. 6-OHDA induced morpholo-
gical and biochemical signs of cell death in DA neurons within
3 h, followed by loss of tyrosine hydroxylase immunoreactive
neurons within 2 days. In substantia nigra (SN) cultures, DA
neurons were much more affected by 6-OHDA than were
GABA neurons. In contrast, DA neurons from the ventral
tegmental area were only lost at higher, non-specific
concentrations of 6-OHDA. The effects of 6-OHDA on nigral
DA neurons were blocked by inhibitors of high affinity DA
transport and by z-DEVD-fmk (150 lM), a caspase inhibitor.
Glial cell line-derived neurotrophic factor (GDNF) treatment
reduced TUNEL labeling 3 h after 6-OHDA exposure, but did
not prevent loss of DA neurons at 48 h. Thus, 6-OHDA can
selectively destroy DA neurons in post-natal cultures of SN,
acting at least in part by initiating caspase-dependent apop-
tosis, and this effect can be attenuated early but not late by
GDNF.
Keywords: apoptosis, caspase, neuroprotection, Parkin-
son’s disease, trophic factor, ventral tegmental area.
J. Neurochem. (2004) 89, 776–787.
Parkinson’s disease is characterized by the progressive
degeneration of dopamine (DA) neurons in the substantia
nigra (SN). Although the cause of this loss is unknown,
evidence suggests a role for oxidative stress (see reviews by
Olanow and Tatton 1999; Stokes et al. 1999). Thus, an
understanding of the mechanisms by which oxidative stress
kills DA neurons and how specific agents can attenuate this
neurodegeneration may provide insights into the etiology and
treatment of the disease. The intracerebral administration of
6-hydroxydopamine (6-OHDA) has been widely used to
cause oxidative stress to DA neurons. Under the right
conditions, this neurotoxin can cause the selective loss of DA
neurons, thereby producing an animal model of certain key
aspects of Parkinson’s disease (reviewed in Zigmond and
Keefe 1997).
6-OHDA also has been widely used to damage DA
neurons in vitro. However, unlike the case for in vivo models,
these in vitro effects of 6-OHDA have never been shown to
be restricted to DA neurons. Indeed, in those cases where it
has been examined, the in vitro effects of 6-OHDA have been
observed to be non-specific (Table 1). As a result, it has been
difficult to draw conclusions regarding the effects of selective
oxidative stress in DA neurons from such studies. Yet, an
Received December 31, 2003; revised manuscript received January 14,
2004; accepted January 16, 2004.
Address correspondence and reprint requests to Michael J. Zigmond,
Department of Neurology, S-526 Biomedical Science Tower, University
of Pittsburgh School of Medicine, Pittsburgh, PA 15213, USA.
E-mail: [email protected] present address of Yun Min Ding is SBRI J-217, MC 2030,
Department of Neurology, University of Chicago, Chicago, IL 60637,
USA.
Abbreviations used: BME, basal medium eagle; DA, dopamine; DAT,
dopamine transporter; DETAPAC, diethylenetriaminepentaacetic acid;
GABA, gamma-amino butyric acid; GDNF, glial cell line-derived
neurotrophic factor; HEPES, N-(2-Hydroxyethyl)piperazine-N¢-(2-ethanesulfonic acid); 6-OHDA, 6-hydroxydopamine; MPTP,
1-methyl-4-phenyl-1,2,5,6-tetrahydropyridine; PBS, phosphate-buffered
saline; SN, substantia nigra; TH, tyrosine hydroxylase; TH+, TH-im-
munostained cells; VTA, ventral tegmental area; z-DEVD-fmk, Z-As-
p(OCH3)-Glu(OCH3)-Val-Asp (OCH3)-fluoromethylketone.
Journal of Neurochemistry, 2004, 89, 776–787 doi:10.1111/j.1471-4159.2004.02415.x
776 � 2004 International Society for Neurochemistry, J. Neurochem. (2004) 89, 776–787
in vitro model of selective DA neuron loss would be of great
benefit in attempts to understand the basis of cell death that
can be triggered by oxidative stress and to develop strategies
for promoting cell survival.
In this report we describe a cellular model in which post-
mitotic, primary DA neurons from the SN are selectively
damaged by 6-OHDA through a process that involves
apoptosis. We then use this model to examine the effects of
glial cell line-derived neurotrophic factor (GDNF), which has
been shown to enhance the survival of developing DA neurons
in culture and protect these neurons from 6-OHDA in vivo.
Materials and methods
Materials
All reagents were of the highest available grade and were purchased
from Sigma/Aldrich (St Louis, MO, USA), unless otherwise noted.
SN neuron culture
All procedures were carried out in accordance with the NIH
Guide to the Care and Use of Animals and approved by the
University of Pittsburgh Animal Care and Use Committee.
Cultures of primary mesencephalic cells were made using the
method of Cardozo (1993) with minor modifications, including
some suggested by Burke, Sulzer and co-workers (Burke et al.
1998). Timed pregnant Sprague-Dawley rats (Hilltop Laboratory
Inc., Scottdale, PA, USA) were housed for 2–5 days and given
free access to water and food under a 12 : 12 h light-dark cycle.
Post-natal pups (P0) were killed during the light phase by
decapitation under aseptic conditions, and brains were removed
from the skulls and placed in cold Gey’s Balanced Salt Solution
(Life Technologies Inc., Grand Island, NY, USA) containing 0.5%
D-glucose. Under a dissecting microscope, a 0.8–1.0-mm thick
coronal section of the mesencephalon was made using a scalpel,
and the regions containing SN were isolated (Fig. 1). Unless
otherwise noted, the regions containing the ventral tegmental area
(VTA) were excluded from the culture. In initial studies, similar
slices were fixed and stained for tyrosine hydroxylase (TH), the
rate-limiting enzyme for DA biosynthesis, to verify the dissected
regions of the midbrain.
Tissue was digested in a solution of papain (15 units/mL,
Worthington Biochemical Corporation, Lakewood, NJ, USA) with
0.45 mg/mL L-cysteine in a dissociation media containing 90 mM
Na2SO4, 30 mM K2SO4, 5.8 mM MgCl2, 0.25 mM CaCl2, 10 mM
Table 1 Summary of selected literature on cytotoxicity of 6-OHDA in vitro
Reference Conclusion Specificity
Age at onset
of culturing
and species
Brain
region
DIV
before
6-OHDA
Exposure
duration
Vehicle
for
6-OHDA
Barkats et al. (2002) 50 lM induced 65%
DA neuron death
– E14 rat Ventral midbrain 3 2 h –
Bronstein et al. (1995) 30 lM damaged DA neurons – E16 rat Ventral midbrain 4–6 48 h 0.1% ascorbate
Cerruti et al. (1993) 10 nM changed DA
cell morphology
– E14 rat Ventral midbrain 2 or 7 48 h Culture medium
Ibi et al. (2001) 100 lM induced 40%
DA cell death
– E16 rat Ventral midbrain 9 24 h Distilled water
Grothe et al. (2000) 100 lM caused 50%
DA cell loss
– E14 rat Ventral midbrain 6 24 h DMEM
Han et al. (2003) 20 lM caused 30–40%
apoptotic loss
of DA cells
– E 14 rat Ventral midbrain 5 6–24 h Ascorbate
Holtz and
O’Malley (2003)
100 lM induced changes
suggesting apoptosis
– E 14 mouse Ventral midbrain 6 6–18 h Ascorbate
Kramer et al. (1999) 10–50 lM caused
widespread cell death
Non-specific E15 rat Ventral midbrain 5 30 min 200 lM ascorbate
Lotharius et al. (1999) 60 lM affected non-DA
neurons
Non-specific E14 CF1
mouse
Ventral midbrain 7 24 h –
Michel and Hefti (1990) 10–100 lM killed DA
and GABA neurons
Non-specific E15 rat Ventral midbrain 6–7 24 h –
Mytilineou and
Danias (1989)
0.1 mM results in greater
toxicity to DA neurons
– E14 rat Ventral midbrain 21 1 h 0.1 mM ascorbate
Pietz et al. (1996) 3 lg/lL induced 40%
DA cell death
– E14 rat Ventral midbrain 7 30 min,
1–24 h
0.2% ascorbate
Rosenberg (1988) 25 lM was non-selective Non-specific E15 rat Cortex 2 48 h –
von Coelln et al. (2001) 40 lM induced 50%
DA cell death
– E14 rat Ventral midbrain 4 24 h –
Effects of 6-OHDA and GDNF on primary SN neurons 777
� 2004 International Society for Neurochemistry, J. Neurochem. (2004) 89, 776–787
HEPES (N-2-hydroxyethylpiperazine)-N¢-(2-ethanesulfonic acid),
0.5% phenol red and 20 mM glucose (pH 7.4) for 1 h at 35�C in a
rotating incubator (Incudrive-S, Schutt Labortechnik, Gottingen,
Germany). After washing twice with dissociation medium, the tissue
was mechanically dissociated with a fire-polished glass Pasteur
pipette in a trituration medium containing 0.1% trypsin inhibitor,
0.1% bovine serum albumin and 10 mM HEPES in basal medium
Eagle (BME; Life Technologies Inc, Carlsbad, CA, USA). To
remove the lighter weight cellular debris, the cell suspension was
collected, layered on top of centrifugation medium containing 1%
trypsin inhibitor and 1% bovine serum albumin in BME and
centrifuged for 4 min at 12.5 g. (GS-6R centrifuge, Beckman
Coulter Inc., Fullerton, CA, USA). The pellet was re-suspended with
trituration medium and cell counts performed with trypan blue to
determine the concentration of dye-excluding, viable cells. The cell
suspension was then adjusted with trituration medium to yield a
concentration of 400 000 cells per mL and 50 lL (20 000 cells) was
added to each well. Culturing was done on glass slides provided
with removable chamber walls that formed 16 wells, each of which
was approximately the size of those on a standard 96-well plate
(0.4 cm2 bottom surface area) (#178599, Nalge Nunc International,
Naperville, IL, USA). The slides were pre-coated with 20 ng/lLpoly D-lysine and 2 ng/lL laminin and contained 200 lL feeding
medium consisting of 0.225% D-glucose, 0.67 mM glutamine,
67 units/mL penicillin, 6.7 mg streptomycin, 0.5% N2 supplement
(Life Technologies Inc.), 2% rat or calf serum (see below) and
10 mM HEPES in BME. Each rat pup produced enough cells for 2–3
wells; thus, a litter of 10–16 pups yielded about 20–32 culture wells
or up to two slides. Cultures were maintained at 37�C in an
atmosphere containing 5% CO2 in equilibrium with H2O.
Rat serum was used in most of our studies. Initial experiments
used commercially produced rat serum. However, rat serum of tissue
culture quality became unavailable from commercial sources during
our studies, prompting us to prepare our own rat serum. For this
purpose, whole blood was collected via cardiac puncture from adult
female rats (generally those that had fostered our pups) killed by
CO2 (Banker and Goslin, 1991) and the blood was kept at 4�C for
24 h followed by centrifugation at 900 g, 4�C, for 10 min. The
supernatant was saved and centrifuged at 20 000 g, 4�C, for 10 min
and the resulting supernatant frozen. Serum prepared in this way
from 10 to 12 rats was then thawed, mixed, aliquoted and stored at
)20�C for up to 12 weeks.
Measurement of breakdown of 6-OHDA under culture
conditions
6-OHDA was dissolved in BME and the solution incubated at 37�Cin an atmosphere maintained at 5% CO2. In an initial series of
experiments, the amount of 6-OHDA remaining in the culture
medium was measured by removing aliquots of solution at several
time points and placing them in a tube containing an equal volume
of 0.1 N HClO3 in order to stop oxidation. Samples then were
analyzed by HPLC coupled with electrochemical detection with
methods for the analysis of DA that we have previously described
(Smith et al. 2002) and employing a 100 lM 6-OHDA standard
made in 0.1 N HClO3 acid to identify the proper peak. The detection
limit of the system was 5 nM. Two to three experiments were
performed for each condition.
Exposure of SN cultures to experimental conditions
Exposure to 6-OHDA was initiated after 3–4 days in vitro (DIV).
Except where noted, the following protocol was employed: Medium
was withdrawn from the wells and replaced with 180 lL BME
without serum followed by the addition of 20 lL of freshly prepared
6-OHDA in vehicle. Vehicle was freshly prepared containing the
metal chelator diethylenetriaminepentaacetic acid (DETAPAC;
10 mM) and ascorbic acid (0.15%, Fisher Scientific, Pittsburgh,
PA, USA) and flushed with N2 for 10 min while the solution was
sitting on ice. Then, a predetermined amount of 6-OHDAwas added
to the vehicle and 20 lL of the 6-OHDA solution or the vehicle
alone was added to the cultures. After 15 min, the medium was
removed, the cultures were gently washed twice with 300 lL BME
plus 10 mM HEPES, 200 lL of feeding medium (described above)
was added to each culture and the cultures were further incubated for
3–48 h at 37�C.
Recombinant human GDNF (100 ng/mL, Upstate Biotechnology,
Lake Placid, NY, USA) was added to the medium in specified
experiments. In those cases where cells were exposed to both GDNF
and 6-OHDA, cultures were pre-treated with GDNF for 1 h prior to
and during exposure to 6-OHDA. Cultures were then gently washed
twice with BME containing 10 mM HEPES, after which feeding
medium containing GDNF was added to the cultures. In studies
attempting to block uptake of 6-OHDA, the DAT inhibitors
nomifensine (10–50 lM) or GBR12909 (2 lM) (Sigma/RBI) were
added 1 h before 6-OHDA exposure and remained until the toxin
was removed and the cultures washed. In studies utilizing the
caspase inhibitor, z-Asp(OCH3)-Glu(OCH3)-Val-Asp (OCH3)-fluor-
omethylketone (z-DEVD-fmk; Enzyme Systems Products, Liver-
more, CA, USA), the inhibitor was dissolved in dimethylsulfoxide
(DMSO) and then 2.5 lL were added to the culture approximately
18 h before exposure to 6-OHDA so as to produce a final
concentration of 150 lM. This z-DEVD-fmk was present in the
cultures during the 6-OHDA exposure procedure and for the 48-h
post-toxin incubation. For the control group, only DMSO was
added.
Fig. 1 Photomicrograph of a coronal section of post-natal rat mes-
encephalon immunostained for tyrosine hydroxylase (TH) after uni-
lateral removal of the SN region. On the left, the entire substantia nigra
(SN) and ventral tegmental area (VTA) are visible and TH-stained cells
appear white against a darker background of unstained tissue. On the
right, TH stained cells of VTA are still apparent, whereas the SN tissue
on this side was dissected for the culture. Scale bar ¼ 500 lm.
778 Y. M. Ding et al.
� 2004 International Society for Neurochemistry, J. Neurochem. (2004) 89, 776–787
Immunocytochemical staining
The cultures were fixed using cold 4% paraformaldehyde in 0.1 M
phosphate-buffered saline (PBS, pH 7.4) for 1 h on ice. Following
several washes of PBS, the cultures were blocked for 30 min in a
blocking solution containing 5% normal donkey serum (Jackson
Immuno-Research, West Grove, PA, USA), 1% bovine serum
albumin and 0.3% Triton X-100 in 0.1 M PBS (pH 7.4), followed by
an overnight incubation at 4�C in blocking solution containing
mouse anti-TH (1 : 1000, Chemicon International, Temecula, CA,
USA) and rabbit anti-GABA (1 : 1000, Sigma/Aldrich). Following
three washes of PBS containing 0.1% Tween-20, the cultures were
incubated in the blocking solution containing Cy-3 (donkey anti-
mouse) and FITC (donkey anti-rabbit) conjugated secondary
antibodies (1 : 200, Jackson Immuno-Research) for 30 min on
ice, followed by staining with Hoechst 33258 reagent (1 : 1000,
Sigma/Aldrich). The chamber walls were then removed and the
slides were coverslipped using Fluoromount-G (Southern Biotech-
nology Associates, Inc., Birmingham, AL, USA) and visualized by
fluorescence microscopy. Staining for TH and GABA were both
negative when the relevant primary or secondary antibodies were
omitted.
Our analysis of the mechanism of cell death included the
measurement of activated caspase-3, typically an executioner
caspase. Rabbit anti-activated caspase-3 (1 : 200, Cell Signaling
Technology, Beverly, MA, USA) was examined using a procedure
similar to that for TH and GABA. Staining for caspase-3 was
negative when the relevant primary or secondary antibodies were
omitted. Double staining for TH and in situ end-labeling of DNA
breaks was achieved by first immunostaining against TH followed
with staining by the method of terminal deoxynucleotidyl transf-
erase (TdT)-mediated dUTP nick end-labeling (TUNEL). The
ApopTag Fluorescein In situ Apoptosis Detection Kit was used
following the instructions provided by the manufacturer (Intergen
Molecular & Cell Biology, Purchase, NY, USA).
Data analysis
The number of positive TH and/or GABA neurons in each well was
counted under 20 · magnification using a Zeiss Axiophot micro-
scope (Carl Zeiss Inc., Germany). Unless otherwise noted, the total
number of TH- or GABA-positive neurons from four random optical
fields was calculated for each culture well. Each of these fields was
1.25 mm in diameter and collectively the four fields represented
approximately 17% of the 0.4 cm2 well. Cells positive for both TH
and TUNEL were identified by counting under 40 · magnification.
Statistical significance was tested using two-way analysis of
variance (Intercooled Stata 7, Stata Corporation, College Station,
TX, USA), followed by multiple comparisons using a Bonferroni
correction. p-values less than 0.05 were considered significant. To
assess the effect of GDNF at 48 h, we used linear contrast to
compare the difference between the means for vehicle control and
6-OHDA-treated samples with the difference between the means for
samples treated with GDNF alone and those treated with 6-OHDA
plus GDNF. Unless otherwise noted, studies were carried out in
triplicate with the means of the three wells being considered a single
number. Such studies were then repeated 3–8 times to produce
means ± SEM. All statistical analyses were then performed on these
untransformed means. However, unless described otherwise, the
values presented in the report are expressed as a per cent of values
obtained from vehicle-treated control cultures. In two experiments,
counting was performed independently by two individuals. We
observed no significant differences (p > 0.9) between the two sets of
counts.
Results
Spontaneous cell death during culturing
DA neurons routinely comprised 5–6% of the total popula-
tion of cells in our SN cultures as defined by immunostaining
for TH at DIV 4 (i.e. 1000–1200 DA cells per 20 000 cells
plated). As will be seen in subsequent figures (e.g. Fig. 3a),
most of these cells displayed multiple, highly branched
processes. The cultures also contained GABA-positive
neurons, which were present in roughly equivalent numbers
to the DA neurons and exhibited a comparable somal size
and degree of process outgrowth. Based on analyses of
cultures from ventral mesencephalon (Michel et al. 1999;
J. D. Jaumotte & M. J. Zigmond, unpublished observations),
we assume that the majority of the remaining cells in the SN
cultures were glia.
The number of TH+ neurons declined over the first 3 days
of incubation. At DIV 2 the number of detectable DA
neurons was about 60% of those present 1 h after plating,
while at DIV 3 and 4 about 40% of DA neurons remained.
Therefore, we selected DIV 4 to begin the remaining studies
as the number of viable DA neurons appeared to plateau at
that time point.
Effect of culture conditions on the response to 6-OHDA
In our initial studies, 6-OHDA was dissolved in BME and
added to cultures, which then were evaluated 48 h later.
Under these conditions, we observed an extensive loss of
both DA and GABA neurons at concentrations of the toxin as
low as 40 lM. Many other cells in the culture also showed
signs of cell death. As 6-OHDA can rapidly oxidize in
solution, we reasoned that the non-specific damage produced
by 6-OHDA was likely due to the action of reactive oxygen
species forming within the culture medium. To test this
hypothesis, 6-OHDA was first dissolved in one of several
different vehicles and incubated in BME (but without the
addition of cells) at 37�C for 5–30 min. We observed that
6-OHDA dissolved in BME alone broke down almost
completely within 5 min. In contrast, when we dissolved
6-OHDA in a vehicle containing BME plus the antioxidant
ascorbic acid (0.15%), the breakdown of 6-OHDA was
significantly slowed such that 82 ± 6.6% of the toxin was
still intact at 20 min (Fig. 2). Further addition of the metal
chelator DETAPAC (1 mM; Berman et al. 1996) followed by
flushing with N2 for 10 min before the addition of 6-OHDA,
further reduced the loss of 6-OHDA during incubation such
that 96 ± 2.0% of the 6-OHDAwas now present after 20 min
Effects of 6-OHDA and GDNF on primary SN neurons 779
� 2004 International Society for Neurochemistry, J. Neurochem. (2004) 89, 776–787
(Fig. 2). Moreover, using this protocol, 6-OHDA (40 lM)
caused a selective and concentration-dependent decline in the
number of DA neurons present 48 h later compared with
cultures exposed to vehicle alone (Fig. 3). For example, after
exposure to 40 lM 6-OHDA, only 47 ± 4.7% (mean ±
SEM) of the DA neurons remained (p < 0.01), whereas
there was no significant loss of GABA neurons (95 ± 3.3%
of control; NS) (Figs 3b and d). At 100 lM 6-OHDA GABA
neurons were reduced to 78 ± 6.4 (p < 0.05); however, this
was significantly less than the loss of DA neurons, which
were reduced to 22 ± 9.5% of control (Figs 3c and d;
p < 0.01). In contrast, 500 lM 6-OHDA, which caused a
near-total loss of DA neurons (3.7 ± 9.2% of control) did
cause a significant loss of GABA cells (41 ± 1.4% of
control; p < 0.01) (Fig. 3d).
Because of these findings, 6-OHDA was dissolved in
vehicle flushed with N2 and containing DETAPAC and
ascorbic acid in all subsequent experiments. However, even
with these precautions, we observed some variability in the
neuronal responses of our cultures to 6-OHDA. For
example, although 100 lM 6-OHDA generally caused a
near total and selective loss of DA neurons, in some cases,
cultures failed to show a loss of DA neurons, whereas
occasionally this concentration of 6-OHDA caused a
significant loss of GABA neurons as well as DA neurons.
Although we are uncertain of the source of this variability,
we hypothesize that it was due primarily to variations in the
amount of actual 6-OHDA present in the culture medium
in any given experiment. Therefore, in each subsequent
study we included wells containing 100 lM 6-OHDA and
used the results of that exposure as an index of the
specificity of the toxin in that particular experiment. Only
when the 100 lM 6-OHDA produced at least a 50% loss of
DA cells and less than a 20% loss of GABA cells did
we proceed with the analysis. This resulted in the exclusion
of approximately 25% of our experiments from further
consideration.
(a) (b)
(c) (d)
Fig. 3 The effects of 15-min exposure to 6-OHDA on the survival of
DA neurons. At DIV 3–4, cultures were exposed to 6-OHDA for
15 min. After 48 h, the cells were fixed and immunostained for TH
(red) and for GABA (green). Representative photomicrographs show
cells incubated with (a) vehicle alone, (b) 40 lM 6-OHDA or (c) 100 lM
6-OHDA. Note the specific loss of DA neurons, but not GABA neurons
in (b) and (c). In (d) data were quantified for 6-OHDA effects on DA
neurons (open bars) and GABA neurons (filled bars) by cell counts of
immunostained neurons. Data represent the mean ± SEM for eight to
10 experiments, performed in duplicate or triplicate. The data were
analyzed by a 2-way analysis of variance and a post-hoc Bonferroni
test on the untransformed data. *p < 0.01 versus control (0 lM 6-
OHDA). Scale bars in a–c ¼ 100 lm.
Fig. 2 6-OHDA degradation as a function of time and different vehi-
cles. Samples were prepared with 6-OHDA (100 lM) in BME alone
(j), BME plus 0.015% ascorbic acid (*), or vehicle containing ascorbic
acid, DETAPAC, and flushed with N2 (m). Samples were incubated for
up to 30 min at 37�C and analyzed by HPLC. Data represent the
mean ± SEM of two to three replicates for each condition.
Fig. 4 The effects of an inhibitor of the high affinity DA transporter on
the toxic effects of 6-OHDA. SN cultures at DIV 3–4 were exposed to
40 lM (open bars) or 100 lM (filled bars) 6-OHDA for 15 min. After
48 h, cultures were fixed and TH+ neurons were counted. DA neurons
treated with 2 lM GBR12909 showed enhanced survival relative to DA
neurons that did not receive GBR12909. Data represent the means
± SEM for five experiments performed in triplicate. The data were
analyzed by a 2-way analysis of variance and a post-hoc Bonferroni
test on the untransformed data. *p < 0.01 for differences between 40
or 100 lM 6-OHDA and 40 or 100 lM + 10 lM GBR12909.
780 Y. M. Ding et al.
� 2004 International Society for Neurochemistry, J. Neurochem. (2004) 89, 776–787
The effect of DAT inhibitors on 6-OHDA-induced
damage
It is generally assumed that the selectivity of 6-OHDA is due
to the specific uptake of the toxin into DA neurons, after
which the 6-OHDA oxidizes to form DA quinone and
reactive oxygen species (see Zigmond and Keefe 1997). This
would be consistent with our observation that specific
damage by 6-OHDA only occurred when care was taken to
prevent the breakdown of 6-OHDA within the culture
medium. To test the assumption that specific damage
required the uptake of 6-OHDA via the high affinity DA
transporter (DAT), we examined the impact of two DAT
inhibitors on the response to 6-OHDA, GBR12909 and
nomifensine. A moderate concentration of GBR12909
(2 lM) completely blocked the damage of DA neurons
normally caused by 40 lM 6-OHDA (p < 0.01) and signi-
ficantly increased the survival of DA neurons from exposure
to 100 lM 6-OHDA (Fig. 4; p < 0.01). Higher concentra-
tions of GBR12909 (‡ 10 lM) were found to be toxic to all
cultured neurons. Likewise, incubation with a low concen-
tration of nomifensine (10 lM) prior to and during exposure
to 100 lM 6-OHDA significantly attenuated the 6-OHDA-
induced loss of DA neurons measured 48 h later without
affecting DA neurons in control cultures. However, this
concentration of nomifensine did not alter the neurotoxic
effects of 100 lM H2O2 or 500 lM 6-OHDA, treatment that
presumably caused non-specific toxicity (data not shown).
Thus, it appeared that the selective effects of 6-OHDA on
DA neurons resulted from an intracellular action of the toxin
subsequent to its uptake through the high affinity DA
transporter.
Comparison of SN with VTA
In vitro studies of DA neurons usually examine cultures
prepared from a large portion of the ventral mesencephalon.
Yet, this area of brain contains at least two groups of DA
neurons, the SN and the VTA. Previous reports suggest that
DA neurons from the SN are more vulnerable to 6-OHDA
than those from the VTA (Hedreen and Chalmers 1972;
Okamura et al. 1995), a finding that parallels the observa-
tion that the SN is much more affected than the VTA in
patients with Parkinson’s disease (Uhl et al. 1985; German
et al. 1989; Hirsch et al. 1997). Therefore, in all of our
studies presented in this report thus far, we had restricted
tissue to the SN region, specifically excluding the VTA. To
determine whether this restriction was necessary, we
compared 6-OHDA-induced toxicity of DA neurons in
cultures prepared from SN with those prepared from VTA.
We observed that DA neurons from the SN were signifi-
cantly more affected by 6-OHDA than were those from the
VTA (Fig. 5). This difference could not be explained in
terms of differences in the density of TH+ cells between SN
and VTA cultures as it persisted even when this density
was equalized through the dilution of VTA cultures with
cells for an adjacent region (Fig. 5b). Therefore, DA
neurons in cultures of the SN appeared to be inherently
more sensitive to 6-OHDA than were DA neurons in
cultures of the VTA.
Contribution of apoptotic cell death to 6-OHDA-induced
DA neuron damage
Having established a specific model for DA neuron death due
to oxidative stress, we next explored the nature of that cell
death. First, we examined the morphology of the DA neurons
3 h after exposure to 6-OHDA. At this time, there was not
yet any reduction in the number of TH+ cells. However,
about half of the DA neurons exposed to a low concentration
of 6-OHDA (40 lM) exhibited fragmented neurites or a
reduction in the number of neurites, as well as a marked
reduction in somal size (Fig. 6a). We also observed immu-
noreactivity for the activated form of caspase-3 in
78 ± 19.6% of the DA cell bodies exhibiting somal shrink-
age (Fig. 6b). This staining was particularly evident in the
34 ± 13.7% of the damaged DA neurons that displayed
condensed nuclei as determined using the Hoechst stain
(Fig. 6c). In addition, 38 ± 21.3% of the DA cells exhibiting
morphological signs of distress also showed positive TUNEL
staining (Fig. 6d; p < 0.001). Caspase-3 activation, con-
densed nuclei and TUNEL labeling were seen at a much
lower frequency in vehicle-treated cultures, and at a much
higher frequency in the DA neurons of cultures exposed to
100 lM 6-OHDA (data not shown).
Finally, we examined the impact of the caspase inhibitor
z-DEVD-fmk on 6-OHDA-induced damage to DA neurons.
Cultures were incubated with z-DEVD-fmk (150 lM) begin-
ning 18 h prior to 6-OHDA exposure and continuing
throughout the experiment. The number of surviving DA
Fig. 5 Effect of 6-OHDA on DA neurons in cultures prepared from SN
and VTA. (a) Equal total numbers of cells from SN and VTA were
exposed to 6-OHDA (40 or 100 lM) for 15 min at DIV 4 and then
examined by immunocytochemistry 48 h later. (b) VTA preparations
were first diluted with tissue dorsal to the VTA in order to approximate
the density of TH+ cells observed in the SN preparations. The
experiment then proceeded as in (a). *p < 0.05 versus control.
Effects of 6-OHDA and GDNF on primary SN neurons 781
� 2004 International Society for Neurochemistry, J. Neurochem. (2004) 89, 776–787
neurons was assessed 48 h after the 15-min exposure to
6-OHDA. The inhibitor completely blocked the DA neuronal
loss typically seen after exposure to 40 lM 6-OHDA and
significantly reduced the effects of 100 lM 6-OHDA (Fig. 7;
p < 0.01). Comparable results have recently been reported
(Han et al. 2003). Collectively, the data suggest that
6-OHDA appears to kill DA neurons in culture through a
caspase-dependant mechanism that is at least partly
associated with apoptosis. Unfortunately, however, the site
of action of z-DEVD-fmk is not entirely clear. The agent was
originally designed to target the asp-glu-val-asp (DEVD) site
on caspase-3, inhibiting activation of the protease. Yet,
though the agent does inhibit caspase-3 (e.g. Masuda et al.
1997), a key executioner protease (Hengartner 2000), it also
is associated with a reduction in the activity of caspase-6, -7,
-8 and -10, albeit at high concentrations (Ki ¼ 500 lM)
(Margolin et al. 1997; Garcia-Calvo et al. 1998).
Impact of GDNF on the survival of DA neurons in
response to 6-OHDA
GDNF has been reported to both protect and rescue DA
neurons from 6-OHDA-induced damage (reviewed by Con-
nor and Dragunow 1998; Bohn 1999) and has recently been
shown to have a ameliorative effect on DA neurons in a
preliminary clinical trial (Gill et al. 2003). We therefore
wished to examine its effects on 6-OHDA-induced toxicity in
our cultures. Fresh GDNF (100 ng/mL) was added to SN
cultures at each of three time points: 1 h prior to, during and
immediately after a 15-min exposure to 6-OHDA. We
observed that 3 h following exposure to 40 and 100 lM
Fig. 6 Effects of 6-OHDA on morphological and cytochemical indices
of apoptosis. Cultures at 3–4 DIV were exposed to 40 lM 6-OHDA for
15 min. Three hours after toxin treatment, cultures were fixed and the
cells were stained using Hoechst reagent, immunostained for TH and
evaluated morphologically for neurite fragmentation and somatal size.
In a representative single culture, triple-labeled cells (arrow heads)
that stained for (a) TH (green) also exhibited neurite fragmentation, (b)
caspase-3 activation (red) and (c) condensed nuclei as revealed by
Hoechst staining (blue). (d) An additional culture treated as in (a–c)
was double labeled for TH and TUNEL. Several DA neurons with
damaged neurites were also TUNEL positive (arrowhead) 3 h after 6-
OHDA (co-labeling for TH and TUNEL appears yellow). All experi-
ments were repeated a minimum of three times. Scale bar ¼ 20 lm
(a–c) or 40 lm (d).
Fig. 7 Effect of z-DEVD-fmk on DA neurons treated with 6-OHDA. SN
cultures exposed to 6-OHDA for 15 min were analyzed 48 h later for
DA neuronal survival by TH immunocytochemistry. SN cultures were
treated with 40 lM (open bars) or 100 lM (filled bars) 6-OHDA plus
DMSO (left bars) or 150 mM z-DEVD-fmk (right bars). Data are
expressed as a percentage of the number of control neurons, and
represent the means ± SEM for five to six experiments, each carried
out in triplicate. *p < 0.01 for differences between 40 lM 6-OHDA and
40 lM + 150 lM z-DEVD-fmk, and between 100 lM 6-OHDA and
100 lM + 150 lM z-DEVD-fmk.
Fig. 8 GDNF effects on DNA fragmentation in DA neurons treated
with 6-OHDA. SN cultures at DIV 3–4 were exposed to 6-OHDA for
15 min and analyzed 3 h later by TUNEL. Control conditions were
compared with 40 or 100 lM 6-OHDA. Cultures either received 100 lM
GDNF 1 h prior to, during and immediately after 6-OHDA or vehicle (+)
or only media changes at comparable times (–). Data represent a
percentage of the mean total number of TH+ neurons that were
TUNEL positive in each well cultured in the presence of the 6-OHDA
vehicle. All means are derived from three to five independent experi-
ments performed in triplicate and counted at 40 · magnification.
*p < 0.01 for differences between cultures receiving 6-OHDA and
those receiving 6-OHDA plus GDNF.
782 Y. M. Ding et al.
� 2004 International Society for Neurochemistry, J. Neurochem. (2004) 89, 776–787
6-OHDA GDNF had markedly attenuated the number of DA
neurons that were TUNEL labeled (Fig. 8; p < 0.01). GDNF
also augmented the total number of TH neurons normally
present 48 h after exposure to 6-OHDA (40 lM). However,
this increase could be attributed to the general effect of
GDNF on DA cell survival that we and others have observed.
Therefore, in the presence of GDNF, 6-OHDA (40 lM)
reduced the number of TH+ neurons to 51 ± 1.1% of control
cultures that also received GDNF alone. This effect was not
significantly different from the effect seen when 40 lM 6-
OHDA was added without GDNF present (53 ± 7.3%)
(Fig. 9). We concluded therefore that whereas GDNF
protected against initial apoptosis caused by 6-OHDA, it
did not protect DA neurons against the longer-term cell death
caused by the toxin.
Discussion
Specificity of the toxic effects of 6-OHDA
We have examined the effects of exposing cultures of
dissociated post-natal cells from the ventral mesencephalon
to 6-OHDA, focusing primarily on cultures from the SN
region. Our initial studies indicated that 6-OHDA caused the
loss of GABA neurons and glia, as well as DA neurons.
These findings are consistent with previous studies using
6-OHDA, in which non-specific damage was observed in
mesencephalic cultures (Michel and Hefti 1990; Bronstein
et al. 1995; Kramer et al. 1999; Lotharius et al. 1999;
Grothe et al. 2000; Zhou et al. 2000), as well as cerebellar
granule neurons (Dodel et al. 1999), cortical cells (Rosen-
berg 1988), thymocytes (Tsao et al. 1996) and microglia
(Takai et al. 1998) (see Table 1). However, we were able to
reduce the non-specific damage produced by 6-OHDA using
five modifications to the standard paradigm: (i) We added
ascorbic acid to diminish the oxidation of 6-OHDA. (ii) We
added the metal chelator DETAPAC, which has been shown
to promote DA uptake into DA terminals in the presence of
ascorbate (Berman et al. 1996). (iii) The medium was
flushed with N2 to reduce dissolved O2 prior to use. (iv)
We limited to 15 min the period during which 6-OHDA was
present and then carefully washed the cells so as to remove as
much of the 6-OHDA as possible from the medium. (v)
Finally, we restricted the source of the DA cells to the SN
region of mesencephalon, excluding cells from VTA, which
would otherwise represent most of the dopaminergic neu-
rons. In the great majority of experiments, this protocol
allowed us to observe a significant amount of 6-OHDA-
induced cell death among nigral DA neurons under condi-
tions in which GABA neurons were unaffected.
The specific effects of 6-OHDA presumably involved its
uptake into DA neurons via DAT and the subsequent
intracellular oxidation of 6-OHDA, as inhibitors of the
transporter blocked toxicity without affecting the non-
specific damage caused by H2O2. These findings are
consistent with the assumption that non-specific damage to
cultured mesencephalic cells caused by 6-OHDA, whether
documented or not, is the result of the non-specific oxidation
of the toxin in the culture medium and the subsequent actions
of reactive oxygen species. Still further complications are
likely to have been introduced into many previous experi-
ments by the failure to separate DA neurons of the SN from
those of the VTA, as the latter appeared to be highly
insensitive to 6-OHDA.
The nature of DA neuron cell death in our model
6-OHDA has been reported to cause the death of DA neurons
by apoptosis, necrosis, or a combination of the two (Marti
et al. 1997; Woodgate et al. 1999; He et al. 2000; Zuch
et al. 2000; Neystat et al. 2001; Han et al. 2003; Holtz and
O’Malley 2003). However, these previous studies have
examined the effects of long exposures of 6-OHDA (> 6 h)
and thus are likely to have measured both specific, intracel-
lular effects of 6-OHDA taken up into DA neurons and non-
specific, extracellular effects of reactive oxygen species
formed in the medium. Under our conditions, 6-OHDA
appeared to produce its specific effects on DA neurons at
least in part through the initiation of apoptosis. This
conclusion is based on four sets of observations. First, 3 h
after exposure to 6-OHDA (40–100 lM), DA neurons in SN
cultures displayed fragmented neurites, shrunken somata and
condensed chromatin. This was followed by a loss of DA
cells 48 h after 6-OHDA exposure. Secondly, we observed
DNA fragmentation at this time as evidenced by nuclear
Fig. 9 The effects of GDNF (100 ng/mL) on the viability of DA neu-
rons exposed to 6-OHDA (40 lM) as assessed 48 h post treatment.
Cultures were treated with 6-OHDA (filled bars) or its vehicle (open
bars). Cultures exposed to GDNF (right pair of bars) received GDNF
for 1 h prior to 6-OHDA, as well as during and after 40 lM 6-OHDA
exposure. The data represents three to five experiments performed in
triplicate. *p < 0.01 for differences between control and 6-OHDA-
treated cultures, and between cultures treated with GDNF and
6-OHDA plus GDNF. Note, however, that 6-OHDA reduced the
number of viable cells by approximately 50% in both the presence and
absence of GDNF.
Effects of 6-OHDA and GDNF on primary SN neurons 783
� 2004 International Society for Neurochemistry, J. Neurochem. (2004) 89, 776–787
fragmentation and positive TUNEL staining. Thirdly, by 3 h
after exposure to 6-OHDA we also detected the activation of
caspase-3, a key executioner protease in the apoptotic
pathway. Fourthly, z-DEVD-fmk, a caspase inhibitor,
blocked the effects of 6-OHDA as measured 48 h after
exposure to the toxin.
The effects of z-DEVD-fmk deserve special attention.
First, this caspase inhibitor also can protect cultured DA
neurons against MPP+ (Bilsland et al. 2002), suggesting a
final common pathway for the death induced by these two
toxins despite several differences observed in the their effects
(e.g. Choi et al. 1999). Secondly, whereas z-DEVD-fmk
prevented 6-OHDA-induced death of DA neurons, the other
indices of cell death – condensed nuclei, TUNEL labeling
and caspase-3 activation itself – were not seen 3 h after
exposure to 6-OHDA in all affected DA neurons. This
suggests either that the onset of these indices of apoptosis
requires more than 3 h to appear, or that not all 6-OHDA-
induced cell death involves conventional apoptotic process
toxicity despite being caspase-dependent.
DA neuron death in Parkinson’s disease
We cannot know whether our 6-OHDA model mimics the
nature of DA neuron death in Parkinson’s disease. The DA
neurons we examined were very young and in culture.
Moreover, the death was triggered by a very brief incubation
to a specific toxin to which patients with Parkinson’s disease
presumably are not exposed, although at least one group has
reported the detection of 6-OHDA in the brains of Parkin-
son’s disease patients (Jellinger et al. 1995). Finally, the
nature of cell death occurring in Parkinson’s disease is still a
matter of controversy. Although oxidative stress is widely
believed to be a key factor in this process, there has been
considerable debate regarding the relative contributions of
apoptosis and necrosis (e.g. see reviews by Burke and
Kholodilov 1998; Graeber et al. 1999; Jellinger 2000;
Hartmann and Hirsch 2001; Graeber and Moran 2002;
Zigmond and Burke 2002). Nonetheless, there are reports at
both the light and electron microscopic level showing
evidence of apoptotic-like morphological and biochemical
changes in the SN of post-mortem material from patients
who suffered from Parkinson’s disease (e.g. Mochizuki et al.
1996; Anglade et al. 1997; Hirsch et al. 1999; Hartmann
et al. 2000, 2001; Tatton 2000). Therefore, we believe it is
reasonable to assume that apoptosis plays a role in the DA
neuron loss that occurs in Parkinson’s disease, and thus that
our in vitro model may be relevant to at least a component of
the pathophysiology of that disease.
Effects of GDNF on 6-OHDA toxicity
The cell death caused by 6-OHDA in our system was altered
by the addition of GDNF. Attention was first drawn to GDNF
as a neuroprotective factor by studies indicating that it
promotes the survival of developing DA neurons in culture
(Engele et al. 1991; Lin et al. 1993). Subsequently, it was
shown that GDNF, as well as vital vectors that contained the
GDNF gene, blocked another kind of DA neuron death – that
which is produced in vivo by 6-OHDA (e.g. Hoffer et al.
1994; Kearns and Gash 1995; Sauer et al. 1995; Tomac et al.
1995; Choi-Lundberg et al. 1997). GDNF also has been
shown to protect against other insults, including lesioning of
motor neurons (Hottinger et al. 2000) and cerebral ischemia
(Miyazaki et al. 1999). Therefore, there is reason to believe
that GDNF can serve as a survival factor in several different
instances.
There also are several studies indicating that GDNF
protects DA neurons from neurotoxins in vitro (Hou et al.
1996; Eggert et al. 1999; Sawada et al. 2000), although
others have reported variable or little protection of cultured
DA neurons (Hou et al. 1997; Kramer et al. 1999). Unfor-
tunately, it is difficult to determine the significance of either
set of observations as, at least in the case of exposure to
6-OHDA, the toxicity may not have been limited to the
dopaminergic cells (see above). Nonetheless, we observed
that GDNF prevented 6-OHDA-induced apoptotic responses
in DA neurons examined 3 h after exposure under conditions
in which we were able to verify the specific effect of the
toxin. We anticipated that these neuroprotective effects of
GDNF would be long lasting, which appears to be the case
in vivo. However, GDNF did not appear to block DA cell
loss as measured after 48 h once the inherent pro-survival
effects of GDNF on control cultures were taken into
consideration. There are several possible explanations for
this discrepancy. For example, the neurotoxic consequences
of 6-OHDA may persist after GDNF or the signaling
mechanism that mediates the effects of GDNF is active.
Alternatively, GDNF may block the apoptosis caused by
6-OHDA, but allow other neurotoxic processes to persist,
processes that were not detected by such measures as nuclear
condensation, TUNEL labeling or caspase activation. Such
processes might normally exist side by side with apoptosis or
only emerge when apoptosis is blocked. It also is possible
that these GDNF-insensitive effects of 6-OHDA are different
from developmental cell death. This would explain the
common observation that GDNF does attenuate the sponta-
neous DA neuron loss normally seen over several days in
culture, even though it did not block the 6-OHDA-induced
cell loss. Finally, GDNF may only delay any given toxic
event rather than block it entirely.
There are some precedents for our finding that GDNF was
ultimately ineffective in blocking toxin-induced cell death.
For example, GDNF (Koeberle and Ball 1998), like BDNF
(Vidal-Sanz et al. 1987), fails to produce a long-term blockade
of retinal ganglion cell death following axotomy. Moreover,
we have recently observed that GDNF blocks some but not all
indices of 6-OHDA-induced cell death in MN9D cells (Ugarte
et al. 2003). In interpreting the significance of the failure of
GDNF to block cell death, it is noteworthy that z-DEVD-fmk
784 Y. M. Ding et al.
� 2004 International Society for Neurochemistry, J. Neurochem. (2004) 89, 776–787
did block the toxic effects of 6-OHDA as measured at 48 h
post exposure to 6-OHDA. Our results may therefore suggest
that GDNF acts upstream of caspase-3. Further investigation
will be necessary to determine the precise nature of the effects
of this trophic factor as well as their biological significance.
Acknowledgements
We thank David L. Cardozo for his invaluable assistance in
establishing our method for ventral mesencephalic cultures, David
Sulzer for helpful discussions regarding culturing and the use of
GDNF, Teresa G. Hastings and Adrian C. Michael for their advice
on reducing the oxidization of 6-OHDA, Sandra M. Pearl for her
participation in the early phase of these studies, Eric A. Falke for his
participation in initial studies comparing SN and VTA neurons,
Susan L. Slagel for performing the analyses of 6-OHDA, Richard J.
Clarke for images prepared in the Center for Biologic Imaging
directed by Simon C. Watkins and Howard E. Rockette, Department
of Biostatistics, for assistance with the statistical analysis, Ruth G.
Perez and Susan D. Giegel for helpful comments on the manuscript,
Emma L. Culligan for preparation of the final draft and Michael E.
Greenberg, in whose laboratory these studies were initiated while
one of the authors (MJZ) was on sabbatical leave. Preliminary
reports of this research have been presented at meetings of the
Society for Neuroscience (New Orleans, LA, November 2000; San
Diego, CA, Nov 2001; Orlando, FL, 2002), the International
Parkinson’s Disease Congress (Helsinki, Finland, July 2001), the
10th meeting of the Israeli Society for Neuroscience (Eliat, Israel,
December, 2001) and Dopamine 2002 (Portland, OR, July 2002).
The research was supported in part by grants from the Scaife Family
Foundation, the National Parkinson Foundation and the USPHS
(NS19608 and NS39267).
References
Anglade P., Vyas S., Javoy-Agid F., Herrero M. T., Michel P. P., Marquez
J., Mouatt-Prigent A., Ruberg M., Hirsch E. C. and Agid Y. (1997)
Apoptosis and autophagy in nigral neurons of patients with Par-
kinson’s disease. Histol. Histopathol. 12, 25–31.
Banker G. and Goslin K., eds. (1991) Culturing Nerve Cells. MIT Press,
Cambridge, MA.
Barkats M., Millecamps S., Bilang-Bleuel A. and Mallet J. (2002)
Neuronal transfer of human Cu/Zn superoxide dismutase gene
increases the resistance of dopaminergic neurons to 6-hydroxy-
dopamine. J. Neurochem. 82, 101–109.
Berman S. B., Zigmond M. J. and Hastings T. G. (1996) Modification of
dopamine transporter function: effect of reactive oxygen species
and dopamine. J. Neurochem. 67, 593–600.
Bilsland J., Roy S., Zanthoudakis S., Nicholson D. W., Han Y., Grimm
E., Hefti F. and Harper S. J. (2002) Caspase inhibitors attenuate
1-methyl-4-phenylpyridinium toxicity in primary culture of
mesencephalic dopaminergic neurons. J. Neurosci. 22, 2637–2649.
Bohn M. C. (1999) A commentary on glial cell line-derived neurotrophic
factor, GDNF. From a glial secreted molecule to gene therapy.
Biochem. Pharmacol. 57, 135–142.
Bronstein D. M., Perez-Otano I., Sun V., Mullis Sawin S. B., Chan J.,
Wu G. C., Hudson P. M., Kong L. Y., Hong J. S. and McMillian M.
K. (1995) Glia-dependent neurotoxicity and neuroprotection in
mesencephalic cultures. Brain Res. 704, 112–116.
Burke R. and Kholodilov N. (1998) Programmed cell death: does it play
a role in Parkinson’s disease? Ann. Neurol. 44, S126–S133.
Burke R. E., Antonelli M. and Sulzer D. (1998) Glial cell line-derived
neurotrophic growth factor inhibits apoptotic death of postnatal
substantia nigra dopamine neurons in primary culture. J. Neuro-
chem. 71, 517–525.
Cardozo D. L. (1993) Midbrain dopaminergic neurons from postnatal rat
in long-term primary culture. Neuroscience 56, 409–421.
Cerruti C., Drian M. J., Kamenka J. M. and Privat A. (1993) Protection
by BTCP of cultured dopaminergic neurons exposed to neurotox-
ins. Brain Res. 617, 138–142.
Choi W. S., Yoon S. Y., Oh T. H., Choi E. J., O’Malley K. L. and Oh Y.
J. (1999) Two distinct mechanisms are involved in 6-hydroxy-
dopamine- and MPP+-induced dopaminergic neuronal cell death:
role of caspases, ROS, and JNK. J. Neurosci. Res. 57, 86–94.
Choi-Lundberg D. L., Lin Q., Chang Y. N., Chiang Y. L., Hay C. M.,
Mohajeri H., Davidson B. L. and Bohn M. C. (1997) Dopamin-
ergic neurons protected from degeneration by GDNF gene therapy.
Science 275, 838–841.
von Coelin R., Kugler S., Bahr M., Weler M., Dichgans J. and
Schulz J. B. (2001) Rescue from death but not from functional
impairment: caspase inhibition protects dopaminergic cells against
6-hydroxydopamine-induced apoptosis but not against the loss of
their terminals. J. Neurochem. 77, 263–273.
Connor B. and Dragunow M. (1998) The role of growth factors in neu-
rodegenerative disorders of human brain. Brain Res. Rev. 27, 1–39.
Dodel R. C., Du Y., Bales K. R., Ling Z., Carvey P. M. and Paul S. M.
(1999) Caspase-3-like proteases and 6-hydroxydopamine induced
neuronal cell death. Brain Res. Mol. Brain Res. 64, 141–148.
Eggert K., Schlegel J., Oertel W., Wurz C., Krieg J. C. and Vedder H.
(1999) Glial cell line-derived neurotrophic factor protects dopam-
inergic neurons from 6-hydroxydopamine toxicity in vitro. Neu-
rosci. Lett. 269, 178–182.
Engele J., Schubert D. and Bohn M. C. (1991) Conditioned media
derived from glial cell lines promote survival and differentiation of
dopaminergic neurons in vitro: role of mesencephalic glia.
J. Neurosci. Res. 30, 359–371.
Garcia-Calvo M., Peterson E. P., Leiting B., Ruel R., Nicholson D. W.
and Thornberry N. A. (1998) Inhibition of human caspases by
peptide-based and macromolecular inhibitors. J. Biol. Chem. 273,
32608–32613.
German D. C., Manaye K., Smith W. K., Woodward D. J. and Saper C.
B. (1989) Midbrain dopaminergic cell loss in Parkinson’s disease:
computer visualization. Ann. Neurol. 26, 507–514.
Gill S. S., Patel N. K., Hotton G. R., O’Sullivan K., McCarter R.,
Bunnage M., Brooks D. J., Svendsen C. N. and Heywood P. (2003)
Direct brain infusion of glial cell line-derived neurotrophic factor
in Parkinson disease. Nat. Med. 9, 589–595.
Graeber M. B. and Moran L. B. (2002) Mechanisms of cell death in
neurodegenerative diseases: fashion, fiction, and facts. Brain
Pathol. 12, 385–390.
Graeber M. B., Grasbon-Frodl E., Abell-Aleff P. and Kosel S. (1999)
Nigral neurons are likely to die of a mechanism other than classical
apoptosis in Parkinson’s disease. Parkinsonism Related Dis. 5,
187–192.
Grothe C., Schulze A., Semkova I., Muller-Ostermeyer F., Rege A. and
Wewetzer K. (2000) The high molecular weight fibroblast growth
factor-2 isoforms, 21,000 mol. wt and 23,000 mol. wt. mediate
neurotrophic activity on rat embryonic mesencephalic dopaminer-
gic neurons in vitro. Neuroscience 100, 73–86.
Han B. S., Hong H. S., Choi W. S., Markelonis G. J., Oh T. H. and Oh Y.
J. (2003) Caspase-dependent and -independent cell death pathways
in primary cultures of mesencephalic dopaminergic neurons after
neurotoxin treatment. J. Neurosci. 23, 5069–5078.
Effects of 6-OHDA and GDNF on primary SN neurons 785
� 2004 International Society for Neurochemistry, J. Neurochem. (2004) 89, 776–787
Hartmann A. and Hirsch E. C. (2001) Parkinson’s disease. The apoptosis
hypothesis revisited. Adv. Neurol. 86, 143–153.
Hartmann A., Hunot S., Michel P. P. et al. (2000) Caspase-3: a vulner-
ability factor and final effector in apoptotic death of dopaminergic
neurons in Parkinson’s disease. Proc. Natl Acad. Sci. USA 97,
2875–2880.
Hartmann A., Troadec J. D., Hunot S., Kikly K., Faucheux B. A.,
Mouatt-Prigent A., Ruberg M., Agid Y. and Hirsch E. C. (2001)
Caspase-8 is an effector in apoptotic death of dopaminergic neu-
rons in Parkinson’s disease, but pathway inhibition results in
neuronal necrosis. J. Neurosci. 21, 2247–2255.
He Y., Lee T. and Leong S. K. (2000) 6-Hydroxydopamine induced
apoptosis of dopaminergic cells in the rat substantia nigra. Brain
Res. 858, 163–166.
Hedreen J. C. and Chalmers J. P. (1972) Neuronal degeneration in rat
brain induced by 6-hydroxydopamine: a histological and bio-
chemical study. Brain Res. 47, 1–36.
Hengartner M. O. (2000) The biochemistry of apoptosis. Nature 407,
770–776.
Hirsch E. C., Faucheux B., Damier P., Mouatt-Prigent A. and Agid Y.
(1997) Neuronal vulnerability in Parkinson’s disease. J. Neural.
Transm. Suppl. 50, 79–88.
Hirsch E. C., Hunot S., Faucheux B., Agid Y., Mizuno Y., Mochizuki H.,
Tatton W. G., Tatton N. and Olanow W. C. (1999) Dopaminergic
neurons degenerate by apoptosis in Parkinson’s disease. Mov.
Disord. 14, 383–385.
Hoffer B. J., Hoffman A., Bowenkamp K., Huettl P., Hudson J., Martin
D., Lin L. F. and Gerhardt G. A. (1994) Glial cell-line derived
neurotrophic factor reverses toxin-induced injury to midbrain
dopaminergic neurons in vivo. Neurosci. Lett. 182, 107–111.
Holtz W. A. and O’Malley K. L. (2003) Parkinsonian mimetics induce
aspects of unfolded protein response in death of dopaminergic
neurons. J. Biol. Chem. 278, 19367–19377.
Hottinger A. F., Azzouz M., Deglon N., Aebischer P. and Zurn A. D.
(2000) Complete and long-term rescue of lesioned adult moto-
neurons by lentiviral-mediated expression of glial cell line-derived
neurotrophic factor in the facial nucleus. J. Neurosci. 20, 5587–
5593.
Hou J. G., Lin L. F. and Mytilineou C. (1996) Glial cell line-derived
neurotrophic factor exerts neurotrophic effects on dopaminergic
neurons in vitro and promotes their survival and regrowth after
damage by 1-methyl-4-phenylpyridinium. J. Neurochem. 66, 74–
82.
Hou J. G., Cohen G. and Mytilineou C. (1997) Basic fibroblast growth
factor stimulation of glial cells protects dopamine neurons from
6-hydroxydopamine toxicity: involvement of the glutathione sys-
tem. J. Neurochem. 69, 76–83.
Ibi M., Sawada H., Nakanishi M., Kume T., Katsuki H., Kaneko S.,
Shimohama S. and Akaike A. (2001) Protective effects of 1 alpha,
25-(OH)(2)D(3) against the neurotoxicity of glutamate and reactive
oxygen species in mesencephalic culture. Neuropharmacology 40,
761–771.
Jellinger K. A. (2000) Cell death mechanisms in Parkinson’s disease.
J. Neural. Transm. 107, 1–29.
Jellinger K., Linert L., Kienzl E., Herlinger E. and Youdim M. B. (1995)
Chemical evidence for 6-hydroxydopamine to be an endogenous
toxic factor in the pathogenesis of Parkinson’s disease. J. Neural
Transm. Suppl. 46, 297–314.
Kearns C. M. and Gash D. M. (1995) GDNF protects nigral dopamine
neurons against 6-hydroxydopamine in vivo. Brain Res. 672, 104–
111.
Koeberle P. D. and Ball A. K. (1998) Effects of GDNF on retinal
ganglion cell survival following axotomy. Vision Res. 38, 1505–
1515.
Kramer B. C., Goldman A. D. and Mytilineou C. (1999) Glial cell line
derived neurotrophic factor promotes the recovery of dopamine
neurons damaged by 6-hydroxydopamine in vitro. Brain Res. 851,
221–227.
Lin L. F., Doherty D. H., Lile J. D., Bektesh S. and Collins F. (1993)
GDNF: a glial cell line-derived neurotrophic factor for midbrain
dopaminergic neurons. Science 260, 1130–1132.
Lotharius J., Dugan L. L. and O’Malley K. L. (1999) Distinct mecha-
nisms underlie neurotoxin-mediated cell death in cultured dop-
aminergic neurons. J. Neurosci. 19, 1284–1293.
Margolin N., Raybuck S. A., Wilson K. P., Chen W., Fox T., Gu Y. and
Livingston D. J. (1997) Substrate and inhibitor specificity of
interleukin-1b-convertin enzyme and related caspases. J. Biol.
Chem. 272, 7223–7228.
Marti M. J., James C. J., Oo T. F., Kelly W. J. and Burke R. E. (1997)
Early developmental destruction of terminals in the striatal target
induces apoptosis in dopamine neurons of the substantia nigra.
J. Neurosci. 17, 2030–2039.
Masuda Y., Nakaya M., Nakajo S. and Nakaya K. (1997) Geranylgera-
niol potently induces caspase-3-like activity during apoptosis in
human leukemia U937 cells. Biochem. Biophys. Res. Commun.
234, 641–645.
Michel P. P. and Hefti F. (1990) Toxicity of 6-hydroxydopamine and
dopamine for dopaminergic neurons in culture. J. Neurosci. Res.
26, 428–435.
Michel P. P., Marien M., Ruberg M., Colpaert F. and Agid Y. (1999)
Adenosine prevents the death of mesencephalic dopaminergic
neurons by a mechanism that involves astrocytes. J. Neurochem.
72, 2074–2082.
Miyazaki H., Okuma Y., Fujii Y., Nagashima K. and Nomura Y. (1999)
Glial cell line-derived neurotrophic factor protects against delayed
neuronal death after transient forebrain ischemia in rats. Neuro-
science 89, 643–647.
Mochizuki H., Goto K., Mori H. and Mizuno Y. (1996) Histochemical
detection of apoptosis in Parkinson’s disease. J. Neurol. Sci. 137,
120–123.
Mytilineou C. and Danias P. (1989) 6-Hydroxydopamine toxicity to
dopamine neurons in culture: potentiation by the addition of
superoxide dismutase and N-acetylcysteine. Biochem. Pharmacol.
38, 1872–1875.
Neystat M., Rzhetskaya M., Oo T. F., Kholodilov N., Yarygina O.,
Wilson A., El-Khodor B. F. and Burke R. E. (2001) Expression of
cyclin-dependent kinase 5 and its activator p35 in models of
induced apoptotic death in neurons of the substantia nigra in vivo.
J. Neurochem. 77, 1611–1625.
Okamura O., Yokoyama C. and Yasuhiko I. (1995) Lateromedial
gradient of the susceptibility of midbrain dopaminergic neurons
to neonatal 6-hydroxydopamine toxicity. Exp. Neurol. 136, 136–
142.
Olanow C. W. and Tatton W. G. (1999) Etiology and pathogenesis of
Parkinson’s disease. Annu. Rev. Neurosci. 22, 123–144.
Pietz K., Odin P., Funa K. and Lindvall O. (1996) Protective effect of
platelet-derived neurons in culture. Neurosci. Lett. 204, 101–104.
Rosenberg P. A. (1988) Catecholamine toxicity in cerebral cortex in
dissociated cell culture. J. Neurosci. 8, 2887–2894.
Sauer H., Rosenblad C. and Bjorklund A. (1995) Glial cell line-derived
neurotrophic factor but not transforming growth factor b 3 prevents
delayed degeneration of nigral dopaminergic neurons following
striatal 6-hydroxydopamine lesion. Proc. Natl Acad. Sci. USA 92,
8935–8939.
Sawada H., Ibi M., Kihara T., Urushitani M., Nakanishi M., Akaike A.
and Shimohama S. (2000) Neuroprotective mechanism of glial cell
line-derived neurotrophic factor in mesencephalic neurons.
J. Neurochem. 74, 1175–1184.
786 Y. M. Ding et al.
� 2004 International Society for Neurochemistry, J. Neurochem. (2004) 89, 776–787
Smith A. D., Amalric M., Koob G. F. and Zigmond M. J. (2002)
Effect of bilateral 6-hydroxydopamine lesions of the medial
forebrain bundle on reaction time. Neuropsychopharmacology
26, 756–764.
Stokes A. H., Hastings T. G. and Vrana K. E. (1999) Cytotoxic
and genotoxic potential of dopamine. J. Neurosci. Res. 55, 659–
665.
Takai N., Nakanishi H., Tanabe K., Nishioku T., Sugiyama T., Fujiwara
M. and Yamamoto K. (1998) Involvement of caspase-like pro-
teinases in apoptosis of neuronal PC12 cells and primary cultured
microglia induced by 6-hydroxydopamine. J. Neurosci. Res. 54,
214–222.
Tatton N. A. (2000) Increased caspase 3 and Bax immunoreactivity
accompany nuclear GAPDH translocation and neuronal apoptosis
in Parkinson’s disease. Exp. Neurol. 166, 29–43.
Tomac A., Lindqvist E., Lin L. F., Ogren S. O., Young D., Hoffer B. J.
and Olson L. (1995) protection and repair of the nigrostriatal
dopaminergic system by GDNF in vivo. Nature 373, 335–339.
Tsao C. W., Cheng J. T., Shen C. L. and Lin Y. S. (1996) 6-Hydroxy-
dopamine induces thymocyte apoptosis in mice. J. Neuroimmunol.
65, 91–95.
Ugarte S. D., Lin E., Klann E., Zigmond M. J. and Perez R. G. (2003)
Effects of GDNF on 6-OHDA-induced death in a dopaminergic
cell line: modulation by inhibitors of PI3 kinase and MEK.
J. Neurosci. Res. 73, 105–112.
Uhl G. R., Hedreen J. C. and Price D. L. (1985) Parkinson’s disease: loss
of neurons from the ventral tegmental area contralateral to thera-
peutic surgical lesions. Neurology 35, 1215–1218.
Vidal-Sanz M., Bray G. M., Villegas-Perez M. P., Thanos S. and Aguayo
A. J. (1987) Axonal regeneration and synapse formation in the
superior colliculus by retinal ganglion cells in the adult rat.
J. Neurosci. 7, 2897–2909.
Woodgate A., MacGibbon G., Walton M. and Dragunow M. (1999) The
toxicity of 6-hydroxydopamine on PC12 and P19 cells. Brain Res.
Mol. Brain Res. 69, 84–92.
Zhou W., Hurlbert M. S., Schaack J., Prasad K. N. and Freed C. R.
(2000) Overexpression of human a-synuclein causes dopamine
neuron death in rat primary culture and immortalized mesenceph-
alon-derived cells. Brain Res. 866, 33–43.
Zigmond M. J. and Burke R. E. (2002) Pathophysiology of Parkinson’s
disease, in Davis, K. L., Coyle, J., Charney, D., Nemeroff, C., eds.
Fifth Generation of Progress, pp. 1781–1794. American College of
Neuropsychopharmacology, Lippincott, Williams & Wilkins,
Philadelphia, PA.
Zigmond M. J. and Keefe K. (1997) 6-Hydroxydopamine as a tool for
studying catecholamines in adult animals: lessons from the
neostriatum, in R. Kostrzewa, ed. Highly Selective Neurotoxins:
Basic and Clinical Applications, pp. 75–108. Humana Press, Inc.
Totawa, NJ.
Zuch C. L., Nordstroem V. K., Briedrick L. A., Hoernig G. R., Granholm
A. C. and Bickford P. C. (2000) Time course of degenerative
alterations in nigral dopaminergic neurons following a 6-hy-
droxydopamine lesion. J. Comp. Neurol. 427, 440–454.
Effects of 6-OHDA and GDNF on primary SN neurons 787
� 2004 International Society for Neurochemistry, J. Neurochem. (2004) 89, 776–787