rac1 inhibition protects against hypoxia/reoxygenation-induced lipid peroxidation in human vascular...
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Vascular Pharmacology 4
Rac1 inhibition protects against hypoxia/reoxygenation-induced lipid
peroxidation in human vascular endothelial cells
Sergio F. Martin a, Subroto Chatterjee b, Narasimham Parinandi c, B. Rita Alevriadou d,*
a Department of Biomedical Engineering, Johns Hopkins University School of Medicine, Baltimore, MD 21205, USAb Lipid Research Atherosclerosis Unit, Department of Pediatrics, Johns Hopkins University School of Medicine, Baltimore, MD 21205, USA
c Davis Heart and Lung Research Institute, Ohio State University College of Medicine, Columbus, OH 43210, USAd Davis Heart and Lung Research Institute and Biomedical Engineering Center, Ohio State University, 473 West 12th Avenue, Columbus, OH 43210, USA
Received 12 November 2004; received in revised form 10 February 2005; accepted 17 May 2005
Abstract
Both in vivo models of ischemia/reperfusion and in vitro models of hypoxia (H)/reoxygenation (R) have demonstrated the crucial role
of the Rac1-regulated NADPH oxidase in the production of injurious reactive oxygen species (ROS) by vascular endothelial cells (ECs).
Since membrane lipid peroxidation has been established as one of the mechanisms leading to cell death, we examined lipid peroxidation
in H/R-exposed cultured human umbilical vein ECs (HUVECs) and the role of Rac1 in this process. H (24 h at 1% O2)/R (5 min)
caused an increase in intracellular ROS production compared to a normoxic control, as measured by dichlorofluorescin fluorescence.
Nutrient deprivation (ND; 24 h), a component of H, was sufficient to induce a similar increase in ROS under normoxia. Either H(24 h)/
R (2 h) or ND (24 h) induced increases in lipid peroxidation of similar magnitude as measured by flow cytometry of diphenyl-1-
pyrenylphosphine-loaded HUVECs and Western blotting analysis of 4-hydroxy-2-nonenal-modified proteins in cell lysates. In cells
infected with a control adenovirus, H (24 h)/R (2 h) and ND (24 h) resulted in increases in NADPH-dependent superoxide production by
5- and 9-fold, respectively, as measured by lucigenin chemiluminescence. Infection of HUVECs with an adenovirus that encodes the
dominant-negative allele of Rac1 (Rac1N17) abolished these increases. Rac1N17 expression also suppressed the H/R- and ND-induced
increases in lipid peroxidation. In conclusion, ROS generated via the Rac1-dependent pathway are major contributors to the H/R-induced
lipid peroxidation in HUVECs, and ND is able to induce Rac1-dependent ROS production and lipid peroxidation of at least the same
magnitude as H/R.
D 2005 Elsevier Inc. All rights reserved.
Keywords: Endothelial cells; Hypoxia/reoxygenation; Nutrient deprivation; Reactive oxygen species; Rac1-regulated NADPH oxidase; Lipid peroxidation
1. Introduction
Reperfusion of ischemic tissue results in the generation
of reactive oxygen species (ROS) that contribute to tissue
injury (Granger and Korthuis, 1995; Grisham et al., 1998;
Zweier et al., 1988). Earlier studies suggested that xanthine
oxidase and the mitochondrial electron transport chain are
important sources of ROS produced during reperfusion
(Acosta and Li, 1979; Ratych et al., 1987; Russell et al.,
1994). However, ROS production by the isolated and
1537-1891/$ - see front matter D 2005 Elsevier Inc. All rights reserved.
doi:10.1016/j.vph.2005.05.002
* Corresponding author. Tel.: +1 614 292 5160; fax: +1 614 292 8778.
E-mail address: [email protected] (B.R. Alevriadou).
continuously ventilated ischemic mouse lungs was shown
to originate from the membrane-associated NADPH oxidase
complex of vascular endothelial cells (ECs) (Al-Mehdi et
al., 1998). ROS production by the membrane-bound
NADPH oxidase in both phagocytic and nonphagocytic
cells is regulated by Rac1, a member of the Rho family of
small GTPases (Abo et al., 1991). The crucial role of the
Rac1-regulated NADPH oxidase in generating the injurious
ROS was demonstrated in an in vivo model of mouse
hepatic ischemia/reperfusion injury, in which the recombi-
nant adenoviral expression of a dominant negative Rac1
(Rac1N17) completely suppressed the ischemia/reperfusion-
induced ROS production and lipid peroxidation and
3 (2005) 148 – 156
S.F. Martin et al. / Vascular Pharmacology 43 (2005) 148–156 149
significantly reduced apoptosis and necrosis in the liver
(Ozaki et al., 2000).
In in vitro models of ischemia/reperfusion, injury due to
exposure of cultured ECs to hypoxia (H)/reoxygenation (R)
was mediated by endogenous ROS production and was a
function of severity of H and duration of both H and R
(McLeod and Sevanian, 1997; Michiels et al., 1992; Terada,
1996). As in the in vivo models, Rac1N17 expression in
cultured human umbilical vein ECs (HUVECs) inhibited the
H/R-induced burst in ROS generation and significantly
reduced cell death, as compared to control cells (Kim et al.,
1998). Peroxidation of the phospholipids in the plasma
membrane mediated by ROS has been established as one of
the mechanisms of cell death (Girotti, 1998). Phospholipid
peroxidation perturbs the integrity of the lipid bilayer of cell
membranes leading to increased plasma membrane perme-
ability and apoptotic cell death (Kriska et al., 2002; Pak et
al., 2002). Exposure of cultured ECs to H/R was shown to
increase both the extent of lipid peroxidation and the number
of apoptotic cells (Li et al., 1998; McLeod and Alayash,
1999; Yang et al., 2001). However, the effect of Rac1 that
regulates the NADPH oxidase-mediated generation of ROS
on the membrane lipid peroxidation in ECs exposed to H/R
has not been reported.
Therefore, in the present study, we investigated the
effect of H/R exposure on lipid peroxidation in cultured
HUVECs and the role of Rac1 in this process. Cells were
exposed to severe prolonged H (24 h at 1% O2) followed
by R up to 2 h. During exposure to H, HUVECs were
maintained in serum-free media, so that they were also
subjected to nutrient deprivation (ND), to create H more
physiologically relevant to ischemia. Since a recent report
has revealed that ND alone is sufficient to induce
production of monocyte chemoattractant protein (MCP)-
1 in ECs that requires ROS generated by the Rac1-
dependent pathway (Lopes et al., 2002), we also
investigated the effect of ND (24 h) on lipid peroxidation
in cultured HUVECs infected either with control adeno-
virus or with adenovirus encoding Rac1N17. The extent
of lipid peroxidation in HUVECs was determined by
flow-cytometric analysis of the intracellular formation of
lipid hydroperoxides using diphenyl-1-pyrenylphosphine
(DPPP), and by Western blotting analysis of the for-
mation of 4-hydroxy-2-nonenal (HNE)-modified proteins
in cell lysates using anti-HNE polyclonal antibodies.
Intracellular generation of ROS was determined by 2V,7V-dichlorodihydrofluorescein diacetate (DCFH-DA)-coupled
flow cytometry. Cellular NADPH oxidase activity was
determined by lucigenin chemiluminescence assay. Our
results showed that H (24 h)/R (5 min–2 h) induces ROS
production and lipid peroxidation mediated by the Rac1-
regulated NADPH oxidase in HUVECs. Our results
further revealed that ND (24 h) is sufficient to induce
lipid peroxidation of similar magnitude as compared to H
(24 h)/R (2 h), which is partially due to Rac1-mediated
ROS production.
2. Materials and methods
2.1. Reagents
tert-Butyl hydroperoxide (tBOOH), cumene hydroper-
oxide (CumOOH), hydrogen peroxide (H2O2), lucigenin,
NADPH, and recombinant (Escherichia coli) human tumor
necrosis factor (TNF)-a were purchased from Sigma
Chemical Company (St. Louis, MO). DCFH-DA and DPPP
were purchased from Molecular Probes (Eugene, OR).
Stock reagents were prepared in medium M199, except
for DPPP that was dissolved in dimethylsulfoxide (DMSO)
at a concentration of 5 mM. Rabbit anti-HNE antiserum was
from Alpha Diagnostic International, Inc. (San Antonio,
TX). Its ability to react with HNE-protein adducts was
demonstrated in immunoblots of homogenates of rat liver
hepatocytes that had been exposed to oxidative stress with
tBOOH (Uchida et al., 1993). Specifically, proteins from
untreated and treated with tBOOH hepatocytes were
subjected to immunoblot analysis in both the absence and
presence of an HNE-peptide competitor. In the presence of
the competitor, the patterns of the unoxidized and oxidized
samples were almost identical and indistinguishable from
the pattern obtained for the control sample in the absence of
competitor, thus proving the specificity of the antibody
reaction.
2.2. EC culture and infection with adenovirus
Cryopreserved primary HUVECs were purchased from
Clonetics (San Diego, CA) and grown in EGM-2 complete
growth medium containing 2% fetal bovine serum (FBS)
and growth supplements (Clonetics). On confluence, cells
were passaged following trypsinization with a 0.05% trypsin
solution (Clonetics). ECs of passages 2 to 8 were used in all
experiments. Both the replication-deficient adenovirus
AdRac1N17, which encodes the myc epitope-tagged dom-
inant-negative allele of Rac1, and the control virus AdhGal,which encodes the inert bacterial LacZ gene, were described
previously (Sulciner et al., 1996; Sundaresan et al., 1995).
Viruses were amplified in HEK-293 cells, purified on
double cesium gradients and plaque-titered (Guzman et
al., 1994). Purified AdRac1N17 and AdhGal had titers of
2�1010 and 5�1010 plaque-forming units (pfu)/ml,
respectively. Some ECs were infected for 48 h before
exposure to H/R or ND (¨80% confluence) at a multiplicity
of infection (MOI) of 150 in EGM-2 complete growth
medium, as described previously (Ng et al., 2002).
2.3. EC treatment with oxidants, H/R or ND
As a positive control for lipid peroxidation, some ECs
were incubated with exogenous hydroperoxides with differ-
ent lipid solubilities, such as tBOOH (0.75 or 1.5 AM),
CumOOH (1 or 4 AM) or H2O2 (0.5 or 5 AM) in M199 for 1
h prior to measurement of ROS production and lipid
S.F. Martin et al. / Vascular Pharmacology 43 (2005) 148–156150
peroxidation. Since the TNF-a-induced signaling pathway
is known to involve intracellular ROS production (Desh-
pande et al., 2000), some ECs were preincubated with TNF-
a at 30 ng/ml in M199 for 1 h. For H/R treatment, ECs in
M199 were exposed to an anoxic gas mixture (95% N2/5%
CO2; Puritan Bennett, Linthicum Heights, MD) in a
humidified incubator (Billups-Rothenburg, Del Mar, CA)
for 2 or 24 h, as described previously (Ng et al., 2002).
Using a Clark-style O2 probe placed in the fluid in the tissue
culture container, the starting partial pressure of oxygen
(PO2) was measured at 150 mm Hg (20% O2) and it dropped
to 10 mm Hg (1% O2) within 15 min of H. Temperature
inside the incubator was maintained at 37 -C with a heating
pad. After H, R was initiated by returning the cells to 95%
air/5% CO2 for 5, 30 min or 2 h. EGM-2 complete medium
was added to the cells right at the onset of R. For ND
treatment, ECs were incubated in M199 in the regular tissue
culture incubator for 24 h. Cell viability was determined by
trypan blue exclusion following normoxia, H/R or ND, and
in each case it was �90%.
2.4. Measurement of ROS and hydroperoxides
To detect the intracellular ROS formation, ECs with and
without adenoviral infection were preloaded with DCFH-
DA (5 AM) in EGM-2 complete medium for 15 min at 37
-C prior to treatment with oxidants, H/R or ND. DCFH-
DA is trapped within cells in the form of DCFH. DCFH is
not fluorescent per se but it is oxidized by potent ROS to
yield measurable fluorescent dichlorofluorescin (DCF)
(Ischiropoulos et al., 1999). To determine the levels of
lipid hydroperoxides, ECs were instead preloaded with
DPPP (200 AM) in EGM-2 complete medium for 15 min
at 37 -C. DPPP reacts stoichiometrically with hydro-
peroxides to give DPPP oxide (DPPP_O), which, due to
its high fluorescence intensity, can be used for determi-
nation of lipid peroxidation in cell membranes (Okimoto et
al., 2000; Takahashi et al., 2001). In either case, after
washing with M199 to remove any extracellular probe,
HUVECs were exposed to stimuli (tBOOH, CumOOH,
H2O2 or TNF-a for 1 h), H (2 or 24 h)/R (5 or 30 min) or
ND (24 h), as described above, following which the cells
were trypsinized, neutralized with trypsin neutralizing
solution (Clonetics) and DCF fluorescence was measured
on a FACScan flow cytometer (Becton Dickinson, San
Jose, CA) with excitation and emission wavelengths set at
475 and 525 nm, respectively. DPPP fluorescence was
measured on a LSRScan flow cytometer (Becton Dick-
inson) with excitation and emission wavelengths set at 350
nm and 400 nm, respectively. For each analysis, 5000
events were recorded.
2.5. Detection of HNE-modified proteins
Following treatment with oxidants, H/R or ND, HUVECs
were scraped into ice-cold lysis buffer consisting of 145 mM
NaCl, 0.1 mM MgCl2, 15 mM HEPES, pH 7.4, 10 mM
EGTA, 1% Triton X-100, 1 mM Na3VO4, and protease
inhibitors such as chymostatin, aprotinin, leupeptin and
pepstatin, each at 10 Ag/ml. Cell extracts were homogen-
ized by sonication and centrifuged at 10,000 rpm for 10
min at 4 -C. Protein concentration in cell lysates was
determined using the bicinchoninic acid assay (Pierce,
Rockford, IL). Supernatant containing 30 Ag of protein was
mixed with 2� sample buffer, boiled for 3 min and applied
in duplicate on 4–20% Tris–glycine gels (Novex, San
Diego, CA) for protein separation by sodium dodecyl
sulfate–polyacrylamide gel electrophoresis (SDS-PAGE) at
100 V constant voltage. One gel was stained with
Coomassie brilliant blue to confirm loading of equal
amount of proteins and the other was used for Western
blotting analysis. For the latter, proteins were electro-
phoretically transferred at 30 V of constant voltage at 4 -Cfor 12 h onto nitrocellulose membranes (Amersham Life
Science, Arlington Heights, IL). Blots were probed with
1:5000 diluted rabbit anti-HNE polyclonal antibody (Alpha
Diagnostic International) and 1:1000 diluted alkaline
phosphatase-conjugated goat anti-rabbit IgG (Calbiochem,
San Diego, CA) and were visualized using the Western-
Breeze\ chemiluminescent Western blot immunodetection
kit (Invitrogen, Carlsbad, CA).
2.6. Measurement of NADPH-dependent O2� production
Following treatment, NADPH-dependent O2� produc-
tion by intact HUVECs was measured using lucigenin-
enhanced chemiluminescence, as described previously (Li
and Shah, 2001). Lucigenin is a compound that emits light
upon interaction with O2� (Gyllenhammar, 1987). Briefly,
ECs were harvested in phosphate-buffered saline (PBS)
and cell pellets were suspended in a balanced salt solution
(130 mM NaCl, 5 mM KC1, 1 mM MgCl2, 1 mM
CaCl2I2H2O, 35 mM H3PO4, and 20 mM HEPES, pH 7.4).
Cell viability determined by trypan blue exclusion was
�90%. HUVEC suspensions were added to duplicate
wells of 96-well plates, followed by NADPH (100 AMfinal concentration) and dark-adapted lucigenin (250 AMfinal concentration). Increases in photon emission were
measured every 60 s for 16 min in a scintillation counter
(Top counter; Packard Instrument, Meriden, CT). A plateau
was achieved after ¨11 min. Light emission (arbitrary
units/min) was first averaged over duplicate wells and then
over the last 5 min in the counter and was normalized by
protein content obtained by a protein assay (bicinchoninic
acid; Pierce). The NADPH-dependent O2� production for
each treatment, a measure of the NADPH oxidase activity,
was estimated by averaging over three independent experi-
ments and expressed as relative lucigenin chemilumines-
cence in mean arbitrary units/min/mg proteinTS.D.
Significant differences between treatments and the corre-
sponding normoxic controls were established by paired t-
test at P <.05.
S.F. Martin et al. / Vascular Pharmacology 43 (2005) 148–156 151
3. Results
3.1. Both H/R and ND increase EC ROS production
ROS generation in HUVECs was monitored using
DCFH-DA and flow cytometry. Exogenously added
H2O2, and organic hydroperoxides (tBOOH and
CumOOH) were chosen as positive controls to show an
increase in intracellular ROS at concentrations and times of
incubation that were previously shown to induce lipid
peroxidation in cell membranes (Okimoto et al., 2000;
Takahashi et al., 2001). From the flow cytometry histo-
grams, it was found that H2O2 (0.5 or 5 AM), tBOOH (0.75
or 1.5 AM) and CumOOH (1 or 4 AM) increased DCF
fluorescence after 1 h of incubation in a dose-dependent
manner (Fig. 1). Stimulation of ECs preloaded with DCFH-
DA with TNF-a at 30 ng/ml for 1 h also resulted in a burst
of intracellular ROS (Fig. 1). H (2 h)/R caused a marginal
increase in DCF fluorescence which was more pronounced
at 5 min from the beginning of R and declined with
progression of R. Prolonged H (24 h)/R was much more
efficient in increasing the DCF fluorescence and, as noticed
under earlier conditions, the signal was greater at 5 min (a
5-fold increase as compared to labeled normoxic control
cells) than at 30 min following R (a 3-fold increase as
compared to labeled normoxic control cells) (Fig. 1). ND
(24 h), a component of the H (24 h) treatment, was alone
sufficient to increase the DCF fluorescence signal by 6-fold
over the labeled normoxic control cells, a level slightly
higher than that due to H (24 h)/R (5 min) (Fig. 1).
Although the cells homogeneously responded by increasing
their intracellular ROS in response to either hydroper-
100 101 102 103 104
100
labeled controlunlabeled control
tBOOH (0.75 µM)tBOOH (1.5 µM)
Fluoresce
100H (2 h)/R (5 min) H (2 h)/R (30 min)
100
Cou
nts
TNF-α (30 ng/ml)ND (24 h)
1
1
1
Fig. 1. Intracellular ROS concentration increases in HUVECs due to exposure to
either exogenously added hydroperoxides (tBOOH, CumOOH, H2O2), TNF-a, H/
to DCF fluorescence distribution (X-axis: DCF fluorescence, Y-axis: number of ce
shown.
oxides, H (2 h) /R or ND (24 h), two cell populations, one
with lower and one with higher fluorescence intensity, were
formed in response to H (24 h) /R (Fig. 1).
3.2. Both H/R and ND increase EC lipid peroxidation
In order to find out if the above treatments increase the
extent of lipid peroxidation, lipid peroxidation was moni-
tored by detection of (a) DPPP fluorescence following
reaction specifically with membrane lipid hydroperoxides
(Okimoto et al., 2000), and (b) HNE, the most prominent
aldehyde generated from hydroperoxides of polyunsaturated
fatty acids that accumulates in cell membranes following
oxidative stress (Esterbauer et al., 1991; Uchida et al.,
1993). When HUVECs preloaded with DPPP were stimu-
lated with either H2O2, tBOOH or CumOOH for 1 h, and
analyzed by flow cytometry, the results showed that
membrane lipid hydroperoxides were formed in a dose-
dependent manner, and tBOOH and CumOOH were more
efficient than H2O2 in causing lipid peroxidation (Fig. 2).
TNF-a, at 30 ng/ml for 1 h, induced a marginal increase in
DPPP fluorescence (Fig. 2). H/R was found to increase the
DPPP fluorescence signal in HUVECs with both times of H
and R. Specifically, H (2 h)/R (30 min) showed no
detectable increase in DPPP fluorescence, whereas H (24
h)/R (2 h) showed a 4-fold increase over the DPPP-
preloaded normoxic control cells (Fig. 2). A two-peak
distribution was evident in the DPPP fluorescence from cells
exposed to H (24 h) /R, indicating that the two cell
populations that raised their intracellular ROS to different
levels also experienced different levels of lipid peroxidation.
ND (24 h) alone caused a 3-fold increase in DPPP
100 101 102 103 104
nce intensity
H (24 h)/R (5 min) H (24 h)/R (30 min)
00CumOOH (1 µM) CumOOH (4 µM)
H2O2 (0.5 µM) H2O2 (5 µM)
00
00
H/R and ND. Cells were prelabeled with DCFH-DA and then exposed to
R or ND, as described in Materials and methods. Histograms corresponding
lls) from one representative experiment out of three with similar results are
104103102101100104103102101100
50
labeled controlunlabeled control
tBOOH (0.75 µM)tBOOH (1.5 µM)
50CumOOH (1 µM)CumOOH (4 µM)
Cou
nts
50H2O2 (0.5 µM)H2O2 (5 µM)
Fluorescence intensity
100
100H (2 h)/R (30 min)H (2 h)/R (2 h)
100H (24 h)/R (30 min) H (24 h)/R (2 h)
TNF-α (30 ng/ml)ND (24 h)
Fig. 2. Membrane lipid peroxidation, as measured by a fluorescent probe, increases in HUVECs following exposure to H/R and ND. Cells were prelabeled with
DPPP before they were stimulated by exposure to exogenously added hydroperoxides (tBOOH, CumOOH, H2O2), TNF-a, HR or ND, as described in
Materials and methods. Histograms corresponding to DPPP_O fluorescence distribution (X-axis: DPPP_O fluorescence, Y-axis: number of cells) from a
representative experiment out of three with similar results are shown.
S.F. Martin et al. / Vascular Pharmacology 43 (2005) 148–156152
fluorescence (Fig. 2), whereas H (24 h) in EGM-2 complete
medium did not show any detectable increase in DPPP
fluorescence (not shown), suggesting that H without ND is
not primarily responsible for inducing lipid peroxidation.
When the formation of HNE-modified proteins was
examined by Western blotting in HUVECs exposed to
different treatments of H/R and ND, it was found that the
intensity of certain bands increased following H/R as
compared to the normoxic control cells in proportion to
the H period alone (Fig. 3). As in the case of DPPP
fluorescence, ND (24 h) alone was sufficient to induce an
accumulation of HNE-modified proteins to at least the same
Fig. 3. Membrane lipid peroxidation, as measured by Western blotting of
HNE-modified proteins, increases in HUVECs following exposure to H/R
and ND. Following cell exposure to different treatments (normoxia, TNF-a,
H/R or ND), the accumulation of HNE-modified proteins was determined
by Western blotting of cell lysates using an anti-HNE polyclonal antibody,
as described in Materials and methods. Data from one representative
experiment out of two with identical results are shown.
magnitude as that caused by H (24 h)/R (2 h) (Fig. 3).
Although TNF-a caused a pronounced increase in densito-
metric intensity of HNE-protein adducts, the band profile
modified by TNF-a was different from that modified by
either H/R or ND (Fig. 3).
Fig. 4. NADPH-dependent O2� production, detected by lucigenin-enhanced
chemiluminescence in intact HUVECs, increases following cell exposure to
H/R and ND. Cells infected with either AdhGal or AdRac1N17 were
exposed to different treatments (normoxia, ND or H/R). Cells were
harvested and distributed in wells of 96-well plates where NADPH and
lucigenin were added, as described in Materials and methods. Light
emission was recorded and expressed as mean arbitrary units/min/mg
protein T S.D. for n =3 independent experiments. The data were analyzed
for statistical significance compared to their corresponding control by
paired t-test: *P <.05, **P <.01.
S.F. Martin et al. / Vascular Pharmacology 43 (2005) 148–156 153
3.3. Both H/R and ND increase the NADPH-dependent O2�
production
Since a phagocyte-type NADPH oxidase is thought to be
a major source of EC ROS (Al-Mehdi et al., 1998;
Mohazzab et al., 1994) and this oxidase generates ROS
following H/R (Kim et al., 1998), we examined if H/R and
ND can each increase the NADPH-dependent O2� produc-
tion by intact HUVECs as measured by lucigenin-enhanced
chemiluminescence. A basal level of lucigenin chemilumi-
nescence even by the normoxic control cells that had been
infected with AdhGal was detected (Fig. 4). Normoxic cells,
either uninfected or infected with the control virus, had the
same level of lucigenin chemiluminescence (not shown). In
ECs infected with AdhGal, ND (24 h) exhibited a 9-fold
increase and H (24 h)/R (2 h) a 5-fold increase, respectively,
compared to the normoxic control (Fig. 4). In cells infected
with AdRac1N17, which results in expression of the
dominant-negative form of Rac1, there was no increase in
lucigenin chemiluminescence following either ND or H/R
treatments, as compared to their corresponding normoxic
control (Fig. 4).
3.4. Rac1-dependent ROS contribute to lipid peroxidation
following either H/R or ND
To examine the role of Rac1-dependent and NADPH
oxidase-generated ROS in the lipid peroxidation following
ND or H/R, the formation of HNE-protein conjugates was
examined by Western blotting in lysates of HUVECs
exposed to ND (24 h) or H (24 h)/R (2 h) following
infection with either the control virus or AdRac1N17.
Although equal amount of protein was loaded for each cell
type based on Coomassie blue staining of the gel, the profile
of HNE-modified proteins was found to be different in
H (2
4 h)/R
(2 h
)
H (2
4 h)/R
(2 h
)
Norm
oxia
Norm
oxia
ND (24 h
)
ND (24 h
)
Mol
. Wt.
(kD)
AdβGal
AdRac1N17
113
5241
92
3529
187
HNE-modifiedproteins
Fig. 5. Rac1 inhibition attenuates the H/R-and ND-induced increases in
membrane lipid peroxidation in HUVECs. Cells infected with either
AdhGal or AdRac1N17 were exposed to different treatments (normoxia,
ND or H/R). The accumulation of HNE-modified proteins was determined
by Western blotting of cell lysates using an anti-HNE polyclonal, as
described in Materials and methods. Data from one representative experi-
ment out of two with identical results are shown.
uninfected cells versus cells infected with the control virus
as compared with cell monolayers exposed to either
normoxia (compare lane 1 of Fig. 3 to lane 1 of Fig. 5),
H/R (compare lane 3 of Fig. 3 to lane 3 of Fig. 5) or ND
(compare lane 5 of Fig. 3 to lane 2 of Fig. 5). Specifically, in
cells infected with the control virus under normoxia, bands
corresponding to ¨70–80 kD HNE-protein adducts appear
more intense compared to uninfected cells under normoxia,
possibly due to redox status changes in cells following viral
infection. In AdhGal-infected cells, ND (24 h) resulted in an
increase in lipid peroxidation at least as large as that
exhibited by cells exposed to H (24 h)/R (2 h) (Fig. 5), as in
the case of uninfected cells (Fig. 3). Rac1 inhibition
significantly reduced the increase in lipid peroxidation due
to either ND or H/R (Fig. 5), suggesting that the ROS
generated by the Rac1-dependent pathway are major
contributors to the ND- and H/R-induced lipid peroxidation.
Similarly, when lipid peroxidation was monitored by DPPP
fluorescence, Rac1 inhibition successfully suppressed both
the ND- and H/R-induced increases in fluorescence (not
shown).
4. Discussion
The present study provides evidence that targeted
inhibition of the small GTPase Rac1, which regulates
ROS production via a membrane-bound NADPH oxidase
(Abo et al., 1991), protects against the H/R-induced lipid
peroxidation in cultured HUVECs. This agrees with
findings from in vivo studies which have revealed that
ischemia-induced lipid peroxidation in perfused rat lungs,
as measured by thiobarbituric acid reactive substances, was
found significantly inhibited by pretreatment with PR-39, a
synthetic peptide that inhibits activity of the lung
endothelial NADPH oxidase by blocking its assembly
(Al-Mehdi et al., 1998). In another study, inhibition of
Rac1 by adenoviral expression of Rac1N17 was shown to
markedly decrease the production of lipid peroxidation
products (malondialdehyde and lipid hydroperoxides) in a
mouse model of hepatic ischemia/reperfusion (Ozaki et al.,
2000). Furthermore, the present study provides evidence
that ND alone, of the same duration as H, is sufficient to
cause at least to the same extent of Rac1-dependent ROS
production and lipid peroxidation as caused by H/R,
suggesting that ND may be more important than H in
activating Rac1 and inducing the production of injurious
ROS by ischemic ECs. In agreement to that, a recent study
has shown that ND rather than H induces the production of
MCP-1 by H/R-exposed cultured human aortic ECs and
MCP-1 production requires a functional Rac1 (Lopes et
al., 2002). In that study, they measured Rac1 activation by
a PAK-affinity precipitation assay and demonstrated that
ND strongly activates Rac1 after 15–30 min and then
induces a prolonged but low level of activation for up to
18 h (Lopes et al., 2002).
S.F. Martin et al. / Vascular Pharmacology 43 (2005) 148–156154
In the present study, we measured the ROS production
by cultured HUVECs at 5 and 30 min from the onset of R,
based on our earlier studies wherein O2� generation was
detected by lucigenin chemiluminescence as early as 5 min
of R (Ng et al., 2002). ND (24 h) alone resulted in at least
as high ROS production as that induced by H (24 h)/R (5
min), when measured by a probe like DCF which is non-
specific to a particular ROS. The existence of two cell
populations (different DCF fluorescence levels) in response
to H (24 h) /R (5 min) may be due to different kinds of
ROS generated by prolonged H (24 h) compared to all
other treatments tested, which, based on their intracellular
distribution and relative reactivity with the trapped DCFH,
result in a two-peak DCF fluorescence distribution. The
NADPH-dependent O2� production by intact ECs is known
to be detectable using lucigenin chemiluminescence,
minimally affected by increasing lucigenin concentration
from 5 up to 400 AM, and is abolished by the flavoprotein
inhibitor diphenylene iodonium suggesting that it can
provide a measure of cellular NADPH oxidase activity
(Li and Shah, 2001). In the present study, ND (24 h)
resulted in higher production of NADPH-dependent O2�, as
measured by lucigenin chemiluminescence, as compared to
H (24 h)/R (2 h). This may be due to additional changes in
Rac1 activity (and resultant NADPH-dependent O2�
production) during the 24 h of H and 2 h of R that are
absent during exposure to ND (24 h under normoxia). The
fact that H/R and ND each generated comparable amounts
of total ROS but different amounts of NADPH-dependent
O2� may be due to activation of other ROS sourecs, such
as xanthine oxidase, cyclooxygenase, phospholipase A2,
endothelial constitutive nitric oxide synthase, the mito-
chondrial (NADH dehydrogenase, cytochrome oxidase)
and the microsomal (cytochrome P-450) electron transport
chains, during the 24 h of H and 2 h of R that are absent
during ND treatment (24 h under normoxia). EC ROS
during H in the absence of ND, in particular, are believed
to originate primarily from the mitochondrial electron
transport chain (Pearlstein et al., 2002). In this study,
functional Rac1 was found to be required for the increase
in NADPH-dependent O2� production due to either ND or
H/R. Although the effect of Rac1 inhibition on the H/R- or
ND-induced increase in ROS production using DCF
fluorescence was not examined, it is known that intra-
cellular ROS levels following H/R or ND are markedly
attenuated in cells either infected with AdRac1N17 (Kim
et al., 1998), pretreated with diphenylene iodonium or
pretreated with the more specific NADPH oxidase inhib-
itor gp91ds-tat (Lopes et al., 2002). This suggests that the
Rac1-regulated NADPH oxidase is a major source of ROS
following H/R or ND. Therefore, ND is primarily res-
ponsible for the production of Rac1-dependent O2� and
total intracellular ROS following H/R, without ruling out
the possibility of independent effects by either H in the
absence of ND or R on Rac1 activation and ROS
production.
The times of detection of lipid peroxidation, 30 min and
2 h after R exposure, were chosen based on the time profile
of lipid hydroperoxide formation as it was monitored by
DPPP_O fluorescence in phorbol ester-stimulated poly-
morphonuclear leukocytes (Okimoto et al., 2000). In order
to show that the extent of DPPP oxidation reflects the extent
of lipid peroxidation within cell membranes, we compared
the reactivities of three hydroperoxides with different
polarities and solubilities with DPPP. Due to its high
lipophilicity, DPPP is supposed to localize within lipid
membranes and react preferentially with lipophilic hydro-
peroxides. H2O2 is highly permeable in the cell membrane
and does not stay within the membrane for long duration to
effectively react with DPPP, hence, the lowest signal
observed among the hydroperoxides tested. CumOOH gave
a higher signal than tBOOH at similar concentrations in
DPPP-labeled U937 cells (Takahashi et al., 2001), but
tBOOH was found to be the most effective stimulus in
DPPP-labeled ECs. No quantitative relationship could be
established between the level of ROS and the resultant
extent of lipid peroxidation. For example, TNF-a resulted in
a markedly greater increase in ROS but a modest increase in
DPPP_O fluorescence. It should be mentioned that
DPPP_O fluorescence provides a cumulative history of
lipid peroxidation of the cell membrane within the course of
the experiment, thus, the signal keeps on amplifying with
time. In addition, it became obvious that the two methods
used to detect lipid peroxidation had different selection
criteria. Thus, TNF-a resulted in a modest DPPP_O
fluorescence signal, but showed a big increase in densito-
metric intensity of certain bands as revealed by the Western
blotting with an anti-HNE antibody. Furthermore, stimula-
tion by TNF-a resulted in increased intensity of different
protein bands containing HNE-adducts as compared to
stimulation by H/R or ND. Both these differences could be
explained if the exact subcellular localization of ROS
following cell exposure to each treatment (as well as the
exact localization of the probe in the case of DPPP) was
known. For example, following stimulation by TNF-a, there
are mitochondrial sources of ROS that are activated
(Deshpande et al., 2000) and this may result in modification
of different proteins by HNE as compared to those modified
due to either H/R or ND. Even viral infection with a control
virus resulted in a different pattern of HNE-protein adducts,
compared to uninfected cells, possibly due to an effect of the
infection itself on the cellular redox status and in agreement
with earlier studies from our group where control infected
cells showed differences in the ROS-mediated profile of
cytosolic tyrosine phosphorylated proteins compared to
uninfected cells (Yeh et al., 1999).
Viability of HUVECs was measured by the trypan blue
exclusion method and was found not to be significantly
affected by H(24 h)/R (2 h with serum readmission) or ND
(24 h). This agrees with other reports which did not find cell
lysis following an overnight exposure of cells to H and an
additional 3 h exposure to R (Mold and Morris, 2001).
S.F. Martin et al. / Vascular Pharmacology 43 (2005) 148–156 155
Contrastingly, some studies showed that either H (16 h)/R (5
min) or ND (24 h) led to ¨30% of cell death (Kim et al.,
1998; Lopes et al., 2002). In the current study, the effect of
different treatments without or with Rac1 inhibition on EC
apoptosis was not examined. However, cellular lipid peroxyl
radicals or lipid hydroperoxides formed in ECs stimulated
by oxidants are known to initiate caspase-3 activation and to
induce an apoptotic signaling pathway (Kotamraju et al.,
2001). One peroxidation product that is involved in the
apoptotic signaling pathway is HNE itself, since it can
activate caspases such as caspase-l, -2, -3 and -8 in human
lens epithelial cells (Choudhary et al., 2002; Herbst et al.,
1999). Based on these findings and also on the fact that
Rac1 inhibition limits the H/R- and ND-induced lipid
peroxidation, it is expected that both H/R and ND will
cause EC apoptosis and Rac1 inhibition will be protective
against apoptosis. Indeed, it has been shown that H (24 h in
complete culture media)/R (3 h) causes ¨30% of human
coronary artery ECs to become apoptotic, as measured by
fragmented DNA end-labeling in situ (Li et al., 1998). ND
during H may further increase apoptosis as revealed by a
study in which bovine aortic ECs exposed to either 48 h of
H in the presence of serum or 48 h of H without serum
exhibited that H plus serum results in ¨15% apoptosis,
whereas H without serum in ¨30% apoptosis (Hogg et al.,
1999). As for the protective effect of Rac1 inhibition on
apoptosis, it was demonstrated that, in an in vivo model of
mouse hepatic ischemia/reperfusion, Rac1N17 expression
significantly suppressed the ischemia/reperfusion-induced
apoptosis in liver (Ozaki et al., 2000).
In summary, H/R induces ROS production and lipid
peroxidation in cultured HUVECs. The Rac1-dependent and
NADPH oxidase-generated ROS are major contributors to
the H/R-induced lipid peroxidation. ND, an integral
component of ischemia, is responsible for most of the H/
R-induced increase in Rac1-dependent ROS production and
resultant EC lipid peroxidation. Thus, targeted inhibition of
the small GTPase Rac1 may be an effective approach in
clinical conditions in which ischemia occurs.
Acknowledgements
We thank K. Irani for the generous gift of AdhGal andAdRac1N17, and A. Kolmakova and S. Deshpande for
technical assistance. This work was supported by National
Institutes of Health grant RO1-HL67027 (B. R. Alevriadou).
S. F. Martin was partially supported by a fellowship from
Ministerio de Educacion y Cultura, Spain.
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