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Review article
Antioxidant and prooxidant mechanisms in the regulation
of redox(y)-sensitive transcription factors
John J. Haddad *
Severinghaus-Radiometer Research Laboratories, Molecular Neuroscience Research Division, Department of Anesthesia and Perioperative Care,
University of California at San Francisco, School of Medicine, Medical Sciences Building S-261, 513 Parnassus Avenue, San Francisco,
CA 94143-0542, USA
Received 2 April 2002; accepted 13 May 2002
Abstract
A progressive rise of oxidative stress due to the altered reduction–oxidation (redox) homeostasis appears to be one of the hallmarks of the
processes that regulate gene transcription in physiology and pathophysiology. Reactive oxygen (ROS) and nitrogen (RNS) species serve as
signaling messengers for the evolution and perpetuation of the inflammatory process that is often associated with the condition of oxidative
stress, which involves genetic regulation. Changes in the pattern of gene expression through ROS/RNS-sensitive regulatory transcription
factors are crucial components of the machinery that determines cellular responses to oxidative/redox conditions. Transcription factors that
are directly influenced by reactive species and pro-inflammatory signals include nuclear factor-nB (NF-nB) and hypoxia-inducible factor-1a
(HIF-1a). Here, I describe the basic components of the intracellular oxidative/redox control machinery and its crucial regulation of oxygen-
and redox-sensitive transcription factors such as NF-nB and HIF-1a.
D 2002 Elsevier Science Inc. All rights reserved.
Keywords: Antioxidant; HIF-1a; NF-nB; Oxygen; Redox; Transcription factors
1. Introduction
Molecular oxygen is an important environmental and
developmental signal that regulates cellular energetics,
growth and differentiation [1–4]. Despite its central role
in nearly all higher life processes, the molecular mecha-
nisms for sensing oxygen levels and the pathways involved
in transducing this information remain largely obscure [1,3].
Oxygen, a gaseous element with colorless, odorless and
tasteless appearance, is the most abundant element on planet
earth, making up about 20% by volume of the atmosphere at
sea level, about 50% of the material of the earth’s surface
and about 90% of water. Biologically, oxygen is necessary
for sustaining the life processes of nearly all living organ-
isms and, chemically, for most forms of combustion. It
readily forms compounds with nearly all other known
elements, except the inert gases, and it is used in blast
furnaces, steel manufacture, chemical synthesis, in resusci-
tation and for many other industrial purposes. Oxygen, then,
is an essential molecule for all aerobic life forms; however,
oxygen plays univalent roles: while oxygen is indispensable
for the cell to obtain the essential chemical energy as a form
0898-6568/02/$ - see front matter D 2002 Elsevier Science Inc. All rights reserved.
PII: S0898 -6568 (02 )00053 -0
Abbreviations: NAC, N-acetyl-L-cysteine; AP-1, activating protein-1;
ASK, apoptosis signal-inducing kinase; ATF, activating transcription factor;
ATP, Adenosine triphosphate; AOP, anti-oxidative potential; ARE, antiox-
idant responsive element; ARDS, adults respiratory distress syndrome;
ARNT, aryl hydrocarbon nuclear translocator; bHLH, basic helix– loop–
helix; BCNU, 1,3-bis-(2-chloroethyl)-1-nitrosourea; BPD, bronchopulmo-
nary dysplasia; BSO, L-buthionine-(S,R)-sulfoximine; BHA, butylated
hydroxyanisole; Cd, cadmium; CREB, cAMP-responsive element binding
protein; CF, cystic fibrosis; JNK, c-Jun N-terminal kinase; DPI, diphenylene
iodonium; EPO, erythropoietin; GLUT, glucose transporter; GSH, L-g-
glutamyl-L-cysteinyl-glycine; GRX, Glutaredoxin; GSSG, glutathione
oxidized disulfide; g-GCS, g-glutamylcysteine synthetase; HO, heme
oxygenase; H2O2, hydrogen peroxide; OH, hydroxyl radical; HOCl,
hypochlorous acid; HIF-1a, hypoxia-inducible factor-1a; InB, inhibitoryprotein; IKK, inhibitory nB kinase; IL, interleukin; LPS, lipopolysacchar-
ide-endotoxin; MAPK, mitogen-activated protein kinase; MT-1, metal-
lothionein-1; NF-nB, nuclear factor nB; NIK, NF-nB inducing kinase;
NLS, nuclear localization signal; NO, nitric oxide; PKA, protein kinase A;
PAS, Per-ARNT-Sim; PDTC, pyrrolidine dithiocarbamate; Redox, reduc-
tion–oxidation; RHD, Rel homology domain; RNS, reactive nitrogen
species; ROS, reactive oxygen species; 1O2, singlet oxygen; O2�S
,
superoxide anion; SOD, superoxide dismutase; TRX, thioredoxin; TNF-a,
tumor necrosis factor-a; TNFR, TNF receptor; VEGF, vascular endothelial
growth factor.* Tel.: +1-415-476-8984; fax: +1-415-476-8841.
E-mail address: [email protected] (J.J. Haddad).
www.elsevier.com/locate/cellsig
Cellular Signalling 14 (2002) 879–897
of ATP, it is often transformed into highly reactive forms,
radical oxygen species (ROS), which are often toxic for the
cell [1,3,5–18]. In order to defend themselves from the
cytotoxic actions of ROS and other free radicals, cells have
acquired multiplicity in endogenous antioxidant systems
during the long evolutionary periods. These defense mech-
anisms include reduction–oxidation (redox) enzymatic sys-
tems such as glutaredoxin and thioredoxin [1–3,19–37].
Studies having the nature of cell biology and molecular
biochemistry have revealed that these molecules are also
involved in cell signaling [1–3,6,15–17,28,33,38–54]. The
term ‘oxidative regulation’ has thus been proposed to
indicate the active role of oxide-reductive modifications of
proteins in regulating their functions. Oxide-reductive reac-
tions of bio-molecules, mostly proteins, formerly considered
as ‘oxidative stress,’ are now considered as ‘signals’ and
contain biological information that is necessary for main-
taining cellular homeostasis [1–3,6,24,28,35,39,55–73].
Altering gene expression is the most fundamental and
effective way for a cell to respond to extracellular signals
and/or changes in its environment, in both the short term and
long term. In the short term, transcription factors are
involved in mediating responses to growth factors and a
variety of other extracellular signals In contrast, the long-
term control of gene expression induced by growth factors
and the changes in gene expression, which occur during
development, are generally (with few exceptions) irreversi-
ble [1,6,17,19,21,24,28,35,50,60,74–105]. During develop-
ment, the expression of specific sets of genes is regulated
spatially (by position/morpho-genetic gradients) and tempo-
rally. Regulation of the signaling responses is governed at the
genetic level by transcription factors that bind to control
regions of target genes and alter their expression. Tran-
scription factors are endogenous substances, usually pro-
teins, which are effective in the initiation, stimulation, or
termination of the genetic transcription process, while in the
cytoplasm, the transcription factor is incapable of promoting
transcription. A signaling event, such as a change of the state
of phosphorylation, occurs, which results in protein subunit
translocation into the nucleus. Transcription is a process in
which one DNA strand is used as a template to synthesize a
complementary RNA. Signal transduction, therefore, in-
volves complex interactions of multiple cellular pathways
[1,2]. In particular, interest in reduction–oxidation/oxygen
(redox{y})-sensitive transcription factors has gained an
overwhelming backlog of interest momentum over the years
ever since the onset of the burgeoning field of free radical
research and oxidative stress. The reason for this is that
redox(y)-sensitive transcription factors are often associated
with the development and progression of many human
disease states; therefore, their ultimate regulation bears
potential therapeutic intervention for possible clinical appli-
cations [9,11,12,17,22,25,37,38,42,47,54,58,69,91,106–
120]. In this review, I will focus on elaborating a compre-
hensive overview of the current understanding of redox/
oxidative mechanisms mediating the regulation of key tran-
scription factors, particularly nuclear factor-nB (NF-nB) andhypoxia-inducible factor-1a (HIF-1a), which regulate a
plethora of cellular functions that span the range from anoxia
and hypoxia to extreme hyperoxia and oxidative stress, both
in physiologic and pathophysiologic conditions.
2. Reduction–oxidation concepts: the paradigm of
oxidative stress
The earliest view of the redox concept is that of the
addition of oxygen molecule (oxidation) to form an
oxidant, or removal of oxygen (reduction) to form a re-
ductant [3,24]. For example, in the burning of hydrogen
(2H2 +O2! 2H2O), the hydrogen is oxidized and the
oxygen is reduced. The combination of nitrogen and
oxygen, which occurs at high temperatures, follows the
same pattern (N2 +O2! 2NO). This formation of NO
oxidizes the nitrogen and reduces the oxygen. In some
reactions, the oxidation process is most prominent. For
example, in the burning of methane (CH4 + 2O2!CO2 +
2H2O), both carbon and hydrogen are oxidized (gain oxy-
gen). The accompanying reduction of oxygen is perhaps
easier to see when the process of reduction is described as the
gaining of hydrogen. On the other hand, the reaction of lead
dioxide at high temperatures appears to be just reduction
(2PbO2! 2PbO +O2). The reduction of PbO2 is clear, but
the associated oxidation of oxygen is easier to see when the
process of oxidation is described as the losing of electrons.
Furthermore, an alternative approach is to describe oxidation
as the loss of hydrogen and reduction as the gaining of
hydrogen. This has an advantage in describing the burning of
methane, for instance. With this approach, it is clear that the
carbon is oxidized (loses all four hydrogens) and that part of
the oxygen is reduced (gains hydrogen). Another alternative
view is to describe oxidation as the losing of electrons and
reduction as the gaining of electrons [3]. Redox concepts are
depicted in a hypothetical overview in Fig. 1.
Today, the idea of free radicals gets a new dimension. Our
human body is more under attack from a free radical-invoked
Fig. 1. An overview of the basic mechanisms mediating reduction–
oxidation (redox) concepts in chemico-biologic interactions.
J.J. Haddad / Cellular Signalling 14 (2002) 879–897880
condition generally referred to as ‘oxidative stress’ [1,5,11–
13,16,17,24,28,33,34,45,50,55,59,94,95,111,114,115,117,1-
21–127]. Each human organ and each human cell is
influenced by oxidative stress, which is separated into
internal (inflammation, autoimmune reactions, dysregula-
tion of metabolism, ischemia) and external (microbiological
organism, electromagnetic radiation, mechanical-, thermal-
and chemical-induced stress) stresses. Oxidative damage
defines the consequences of a mismatch between the pro-
duction of the reactive oxygen and nitrogen species (ROS/
RNS) and the ability to defend against them. For the most
part, ROS/RNS originate in the body; they are numerous
and include free radicals such as superoxide (O2� ), nitric
oxide (NO) and hydroxyl ion (OH), as well as the oxygen-
derived species such as singlet oxygen (1O2), hydrogen
peroxide (H2O2) and hypochlorous acid (HOCl) (Fig. 2)
[1,3,4,7,16,20,24,42,78]. Major sources of ROS/RNS
include, but are not exclusive to, mitochondrial oxidative
metabolism, phospholipid metabolism and proteolysis. Bio-
logical systems are protected from the threat of oxidative
assault by a diversity of mechanisms designed to suppress
pernicious oxidative pathways. Raised against the challenges
are an extensive and highly effective array of protective
agents and defense antioxidant mechanisms. These comprise
numerous small molecular weight antioxidants to forestall
initiation of oxidative damage and/or limit its propagation,
enzymes that convert and detoxify ROS/RNS, enzymes to
repair oxidative damage when it occurs and mechanisms to
route damaged molecules for destruction and replacement
[10,17,18,20,22,25,26,28,33,54,79,87,119,120,127–138].
For mitochondria where reactive intermediates inevitably
leak from the electron transport chain to cause local damage,
rapid turnover and replacement of the organelle is crucially
recognized. In fact, the need for rapid regeneration of
mitochondria is often used to explain its independent store
of DNA; lastly, outer segments have a turnover mechanism
based on disc renewal and shedding to supplement local
repair [1,2,4,24,139]. Antioxidant processes usually work by
direct scavenging of the initiating prooxidant species. Each
tissue, for instance, has an anti-oxidative potential (AOP),
which is determined by the balance and those exerting an
enzymatic and non-enzymatic antioxidants to indicate a need
for such protection. A healthy cell is one in which the
antioxidant systems effectively keep the level of prooxidants
below a critical, non-pernicious threshold. ROS/RNS rad-
ical pathways and their enzymatic dismutation are shown
in Fig. 3.
3. Oxygen radicals and redox regulation of NF-KB
signaling
3.1. The Rel/NF-jB family: an overview
To accommodate an ever-changing microenvironment,
cells adjust the pattern of gene expression by adaptive
regulation of a host of transcription factors, which bind their
respective cognate sites in the regulatory elements of targeted
genes (Fig. 4) [1,2,91,140]. The recognition of ROS/RNS
and redox-mediated protein modifications as transducing
signals has opened up a new field of cell regulation and
provided a novel way of controlling disease processes. One
such approach has been proven feasible for gene expression
governed by the transcription factor NF-nB. The nature of
the redox/oxidative mechanisms mediating the regulation of
NF-nB, as a typical example of tightly controlled cellular
signaling, will be thoroughly discussed here.Fig. 2. The oxygen triangle and the various associated free radicals
emanating from its corners.
Fig. 3. Selective dismutation of reactive oxygen (ROS) and nitrogen (RNS)
species, representing a schematic model of the pathways leading to the
generation of ROS/RNS. A number of major cellular enzymes that defend
against oxidative stress have been conserved through evolution. Superoxide
(O2� ) anion is metabolized via the dismutation reaction 2O2
� +
2H + !O2 +H2O2, which is catalyzed by superoxide oxidoreductase
dismutase (SOD), a cytoplasmic enzyme that is constitutively expressed,
and a mitochondrial enzyme that is induced in response to oxidant stress.
The H2O2 produced by the dismutation of O2� is converted by one pathway
to H2O and O2 by catalase (CAT) in peroxisomes and by glutathione
peroxidase (GSH-PX) in the cytoplasm, at the expense of reduced
glutathione (GSH), leading to the formation of oxidized glutathione
disulphide (GSSG) that is recycled back to GSH by glutathione reductase
(GSSG-RD). H2O2 could be further converted by another pathway
involving iron into hydroxyl radical (OH), an injurious ROS causing
cellular damage. This iron-catalyzed reaction, known as the Fenton-like
reaction, is impeded by the iron chelator desferrioxamine (DSF), which is
also capable of neutralizing the toxicity of OH.
J.J. Haddad / Cellular Signalling 14 (2002) 879–897 881
Although the transcription factor NF-nB has been orig-
inally recognized in regulating gene expression in B-cell
lymphocytes [49], subsequent investigations have demon-
strated that it is one member of a ubiquitously expressed
family of Rel-related transcription factors that serve as
critical regulators of many genes, including those of pro-
inflammatory cytokines [6,21,28,40,55,63,65,74,76,86–
89,91,94,121,133,134,140–163]. NF-nB comprises the Rel
family of inducible transcription factors that are key media-
tors in regulating the progression of the inflammatory process
[2,35,39,40,44,63,65,82–84,87,91,94,95,111,132,141,164–
166]. Therefore, activation and regulation of the NF-nB/Reltranscription family, via nuclear translocation of cytoplas-
mic entities and complexes, play a central role in the
evolution of inflammation through the regulation of genes
essentially involved in encoding pro-inflammatory cytokines
and other inflammatory mediators [167]. The NF-nB/Relfamily includes five members: NF-nB1 (p50/p105 {p50
precursor}), NF-nB2 (p52/p100 {p52 precursor}), RelA
(p65), RelB (p68) and c-Rel (p75) [63,92,148,158,168–
172]. Despite the ability of most Rel members (with the
exception of p68) to homodimerize, as well as to form
heterodimers, with each other, the most prevalent activated
form of NF-nB is the heterodimer p50–p65, which possesses
the transactivity domains necessary for gene regulation
(Fig. 5). The NF-nB members contain a Rel homology
domain (RHD), which is responsible for dimer formation,
nuclear translocation, sequence-specific consensus DNA
recognition and interaction with inhibitory-nB (InB) pro-
teins, which are the cytosolic inhibitors of NF-nB. The
translocation and activation of NF-nB in response to various
stimuli are sequentially organized at the molecular level. In
resting, unstimulated cells, NF-nB resides in the cytoplasm as
an inactive NF-nB/InB complex, a mechanism that hinders
the recognition of the nuclear localization signal (NLS) by
the nuclear import machinery, thereby retaining the NF-nBcomplex within the cytosol. In its inactive state, the hetero-
dimeric NF-nB, which is mainly composed of two subunits,
p50 (NF-nB1) and p65 (RelA), is present in the cytoplasm
associated with InB. Upon stimulation, such as with cyto-
kines and lipopolysaccharide-endotoxin (LPS), derived from
the cell wall of Gram-negative bacteria, InB-a, the major
cytosolic inhibitor of NF-nB, undergoes phosphorylation on
serine/threonine residues, ubiquitination and subsequent pro-
teolytic degradation, thereby unmasking the NLS on p65 and
allowing nuclear translocation of the complex (Fig. 5). This
sequential propagation of signaling ultimately results in the
release of NF-nB subunits from InB-a inhibitor, allowing
translocation and promotion of gene transcription. Signals
emanating from membrane receptors, such as those for IL-1
and TNF-a, activate members of the MEKK-related family,
including NF-nB-inducing kinase (NIK) and MEKK1, both
of which are involved in the activation of InB kinases, IKK1
and IKK2, components of the IKK signalsome [50,63,
78,87,112,143,145,148,150,173–177]. These kinases phos-
phorylate members of the InB family, including InB-a, themajor cytosolic inhibitor of NF-nB, at specific serines withintheir amino termini, thereby leading to site-specific ubiquiti-
nation and degradation by the proteasome (Fig. 5). This
sequential trajectory culminating in the inducible degradation
of InB, which occurs through consecutive steps of phosphor-ylation and ubiquitination, allows freeing of the NF-nBcomplex, which translocates to the nucleus to bind specific
nB moieties and initiate gene transcription (Fig. 6).
Rel/NF-nB transcription factors are a family of structur-
ally related eukaryotic transcription factors that are involved
in the control of a vast array of processes, such as immune
and inflammatory responses, developmental processes, cel-
lular growth and programmed cell death (apoptosis). In
addition, these factors are active in a number of disease
states, including cancer, arthritis, inflammation, asthma,
neurodegenerative diseases and cardiovascular abnormal-
ities [10,17,25,38,44,55,58,69,91,95,112,113,166,178]. The
immunoregulatory approach aimed at targeting the NF-nB
Fig. 5. Transcriptional regulation of NF-nB and the structures of the Rel
family transcription factors. Shown are the generalized structures of the two
classes of Rel transcription factors. All have a conserved DNA-binding/
dimerization domain called the Rel homology (RH) domain, which also has
sequences important for nuclear localization (N) and InB inhibitor binding.
Class I proteins have additional inserted sequences in the RH domain. The
C-terminal halves of the class I Rel proteins have ankyrin repeat-containing
inhibitory domains, which can be removed by proteasome-mediated
proteolysis (Protease). The C-terminal halves of the class II Rel proteins
have transcriptional activation domains.
Fig. 4. Gene transcriptional overview implicating selective transcription
factor–DNA complex interactions.
J.J. Haddad / Cellular Signalling 14 (2002) 879–897882
signaling pathway, therefore, remains of particular interest.
Since NF-nB regulates host inflammatory and immune
responses by increasing the expression of specific genes
and enzymes whose products contribute to the pathogenesis
of the inflammatory process, selective modulation of this
transcription factor bears a typical therapeutic approach for
the control and regulation of inflammatory-associated dis-
eases. Unfortunately, due to convergence of more than one
mechanism upon the onset and progression of the inflam-
matory process, which regulates NF-nB signaling, it has
been extremely difficult solely to target this pathway with-
out affecting other cellular functions. The myriad of genes
directly targeted by NF-nB is given in Table 1.
3.2. Oxidative stress-mediated regulation of NF-jB
What are the signaling cofactors that trigger and mediate
NF-nB signaling cascades? Not much is known about what
exactly happens immediately downstream of cell surface
receptors. The expression of genes in response to trans-
ducing signals from surface receptors is predominantly
determined by the conditions of the cell microenvironment.
Prime examples of such regulation are found in embryonic
development of all multicellular organisms [24,25,179]. The
naturally occurring regulating agents, for example, interact
with specific receptors, which subsequently transduce a
signal onto the nucleus for the regulation of gene expression
and activation. The putative oxygen sensor responds to
dynamic variation in pO2. Upon ligand binding, this mem-
brane-bound receptor transduces intracellular chemical/
redox signals that relay messages for the regulation of gene
expression, a phenomenon mainly involving the activation
of transcription factors (Fig. 6) [6,17,28,50,149,179,180].
NF-nB is among the most important transcription factors
shown to respond directly to oxidative stress [6,8,15,28,55,
68,70,73,74,76,77,118,121,160,174,179,181–183]. Antiox-
idants, for instance, have been reported to block NF-nBactivation in certain cell types, leading to the hypothesis
that the activation of this transcription factor is mediated
by ROS in response to specific stimuli [10,28,35,36,50,70,
71,95,133,134,136,137,140,144,145,153,159,173,177,184].
The involvement of ROS is postulated to regulate and
modulate the activity of the upstream kinases that converge
onto the NF-nB signaling activation pathway. In this respect,
wide arrays of antioxidants that can detoxify ROS/RNS have
been reported to suppress the activation of NF-nB, suggest-ing a key role for reactive species in NF-nB signaling. For
instance, hepatocarcinogen 2-acetylaminofluorene treat-
ments led to the increase of intracellular ROS, which caused
Table 1
Direct NF-nB target genes
Cytokines/Growth factor
Interleukin (IL)-1a, IL-1h, IL-2, IL-3, IL-6, IL-8, IL-12, Tumor Necrosis
Factor (TNF)-a, Lymphotoxin (LT)-a, Interferon (IFN)-h, GranulocyteColony-Stimulating Factor (G-CSF), Macrophage Colony-Stimulating
Factor (M-CSF), Granulocyte-Macrophage Colony-Stimulating Factor
(GM-CSF)
Cytokine receptors
IL-2 Receptor a-Chain (IL-2Ra)
Stress proteins
Serum Amyloid A Protein (SAA), complement factors B, C3 and C4, a1-
Acid Glycoprotein
Adhesion molecules
Intracellular Adhesion Molecule 1 (ICAM-1), Vascular Cell Adhesion
Molecule 1 (VCAM-1), Mucosal Addressin Cell Adhesion Molecule 1
(MAdCAM-1), E-Selectin
Immunoregulatory molecules
Immunoglobulin n Light Chain (Ign), Major Histocompatibility complex
(MHC class I and II), T-Cell Receptor (TCRa and h), h2-Microglobulin,
Invariant Chain (Ii), Transporter Associated with Antigen Processing
(TAP-1), Proteasome Subunit (LMP-2), Inducible Nitric Oxide Synthase
(iNOS), Inhibitory nB (InB), p53
Fig. 6. Rel/NF-nB signal transduction. Various signals converge on
activation of the InB kinase (IKK) complex. IKK then phosphorylates InBat two N-terminal serines, which signals it for ubiquitination and proteolysis.
Freed NF-nB (p50-RelA) enters the nucleus and activates gene expression.
The activation of NF-nB is thought to be part of a stress response as it is
activated by a variety of stimuli that include growth factors, cytokines,
lymphokines, UV, pharmacological agents, and stress. In its inactive form,
NF-nB is sequestered in the cytoplasm, bound by members of the InB family
of inhibitor proteins, which include InB-a, InB-h, InB-g and InB-q. Thevarious stimuli that activate NF-nB cause phosphorylation of InB, which is
followed by its ubiquitination and subsequent degradation. This results in
the exposure of the nuclear localization signals (NLS) on NF-nB subunits
and the subsequent translocation of the molecule to the nucleus. In the
nucleus, NF-nB binds with a consensus sequence (5V-GGGACTTTCC-3V) ofvarious genes and thus activates their transcription.
J.J. Haddad / Cellular Signalling 14 (2002) 879–897 883
the activation of IKK kinases, the degradation of InB-h and
the accumulation of NF-nB in the nuclear compartment
[147]. Similarly, a-phenyl-tert-butylnitrone, an effective
spin-trapping agent that reacts with and stabilizes free radical
species, has been shown to inhibit pancreatic h cell death and
the development of insulin-dependent diabetes mellitus in an
NF-nB-dependent pathway [35,133,134,153]. Furthermore,
superoxide dismutase (SOD) expression has negative effects
on the activation of NF-nB in transient focal cerebral
ischemia, indicating the involvement of specific ROS
[173]. Of interest, treatment of mammalian cells with H2O2
induced the nuclear translocation of NF-nB and its binding to
nB DNA sequences present in the promoter region of
numerous genes. The role of selenium in NF-nB activation
was analysed in human T47D cells over-expressing the
seleno-dependent detoxifying enzyme glutathione peroxi-
dase [182]. Following exposure to H2O2, these cells showed
a seleno-dependent decreased accumulation of intracellular
ROS and NF-nB activation. This phenomenon was corre-
lated with an inhibition of the nuclear translocation of NF-nB(p50 subunit) and with an absence of InB-a degradation. It
was also reported that the half-life of InB-a in untreated cells
was increased two-fold by the overexpression of the active
glutathione peroxidase. These results suggest that selenium
is a key element that, through its modulation of glutathione
peroxidase activity, can inhibit NF-nB and can up-regulate
cytosolic InB-a normal half-life [182]. In addition, an
impaired pulmonary NF-nB activation has been observed
in response to LPS in NADPH oxidase-deficient mice [156].
Of note, xanthine oxidase-derived ROS can activate NF-nB[185] and cellular enrichment with polyunsaturated fatty
acids can induce the development of oxidative stress con-
dition and the activity of activating protein-1 (AP-1) and NF-
nB [72]. Furthermore, hyperoxia has been reported to up-
regulate the nitric oxide (NO)-sensitive pathway in vitro and
similarly activate AP-1 and NF-nB, suggesting a role for
RNS [186].
Because NF-nB can be rapidly induced in a variety of
cell types by a diverse set of seemingly unrelated agents, it
has been proposed that agents activating this transcription
factor do so by increasing a minimum intracellular effective
oxidative stress threshold [14,55,73,96,126,160,186]. A
novel recent study by Blackwell et al. [76] has highlighted
the significance of oxidative stress in regulating NF-nB.Although in vitro data has linked ROS to the activation of
NF-nB, little information exists regarding this relationship
in human disease. It was hypothesized that bone marrow
transplantation (BMT), for instance, would impart a degree
of oxidative stress that might lead to the in vivo activation of
NF-nB. Because NF-nB regulates transcription of proin-
flammatory mediators, it was reasoned that the activation of
NF-nB might contribute to the development of transplant-
related complications. To evaluate NF-nB activation in
humans, Blackwell and colleagues measured NF-nBDNA-binding activity in nuclear extracts of bronchoalveolar
lavage (BAL) cells obtained before and after allogeneic
BMT. Changes in BAL cells NF-nB activation were com-
pared with changes in urinary F2-isoprostane concentration,
an indicator of in vivo free radical-catalyzed lipid perox-
idation. Although the extent of the in vivo lipid peroxidation
has substantial inter-individual variability over time, it was
found that there was a strong correlation between the pre/
post-BMT ratio of urinary isoprostane concentrations and
pre/post-BMT ratio of NF-nB binding activity in BAL cells.
Although limited by the small number of patients studied,
this data closely linked oxidative stress to NF-nB activation
in human alveolar macrophages following BMT. It is
possible that such interactions may contribute to the clinical
course after BMT by affecting the transcription of proin-
flammatory genes [76]. On the oxidative mechanisms that
mediate the regulation of NF-nB, the effect of pyrrolidine
dithiocarbamate (PDTC), which potently blocks the activa-
tion of NF-nB in serum-exposed conditions by reducing
ROS [15,183], was explored on the activation of MAPKs
[144]. PDTC transiently increased the phosphotransferase
activity of c-Jun N-terminal kinase-1 (JNK-1), which in turn
activated the transcriptional activity of AP-1. The activation
of JNK was completely decreased in dominant negative
JNK-1 transfected cells and the PDTC-induced cell death
was attenuated in these cells. In addition, AP-1 activation
was decreased in the JNK-1 transfected cells, compared
with vector-transfected cells. The NF-nB inhibitor also
transiently activated MAPKp38 but its inhibition did not
affect the regulatory effect on PDTC-induced cell death,
suggesting that oxidative stress-induced cell death is medi-
ated by MAPKJNK and not by MAPKp38. Furthermore, it
has been reported that the tumor necrosis factor receptor
(TNFR) is implicated in ROS-mediated regulation of NF-nBand its involvement in creating balance between pro- and
anti-apoptotic signaling cofactors governing cell fate in
oxidative stress [56,78]. In accordance with the aforemen-
tioned observations, a cytokine-responsive upstream InBkinase has been found to initiate a ROS-dependent activa-
tion of the NF-nB signaling pathway, suggesting the
involvement of selective kinases in cytokine-mediated NF-
nB regulation [148,177]. Similarly, the involvement of NF-
nB in cardiomyocyte hypertrophy requires the activation of
apoptosis signal-regulating kinase-1 (ASK-1) in a G-pro-
tein-dependent pathway, which was postulated to allow the
induction of intracellular ROS [165]. Of note, it has been
reported that the cooperativity between oxidants and TNF-a
in the activation of NF-nB requires the involvement of a
Ras/Rac/MAPK-dependent mechanism [161,174,181,187].
Moreover, the mitochondria-derived ROS have been
observed as crucial mediators in the regulation of NF-nB[188]. For instance, it was found that the activation of NF-
nB by TNF-a was blocked by rotenone or amytal, inhibitors
of complex I of the mitochondrial respiratory chain [189].
On the other hand, antimycin A, an inhibitor of complex III,
enhanced TNF-a activation of NF-nB, indicating a key role
of mitochondria-derived ROS in mediating NF-nB signaling
[81,189]. Furthermore, g-glutamyl-transpeptidase (GGT), a
J.J. Haddad / Cellular Signalling 14 (2002) 879–897884
key enzyme implicated in the homeostasis of intracellular
reduced GSH, and hence in the regulation of the cellular
redox state, has been implicated in the extracellular cleavage
of GSH and the generation of ROS. Using a model cell line,
the V79 GGT, which highly expresses a human GGT
transgene, GGT-induced oxidant stress was shown to mod-
ulate intracellular transcription factors. GGT-dependent
ROS production induced the NF-nB-binding and transacti-
vation activities [19]. This induction mimicked the one
observed by H2O2 and was inhibited by catalase, suggesting
the involvement of H2O2 in the NF-nB activation.
However, the model of ROS/RNS (oxidative stress) as
exclusive messengers in the regulation of the NF-nB signal-
ing pathway cannot be universally accounted for (Fig. 7)
[16,24,121,142,175,190–192]. For instance, Ginis and col-
leagues [193] reported that ROS could act synergistically
with TNF-a in causing cytotoxicity via the inhibition of a
cytoprotective branch of TNF-a signaling pathways, which
starts with NF-nB activation. Furthermore, addition of
glucosamine to rat chondrocytes treated with IL-1h or with
ROS decreased the activation of NF-nB, but not that of AP-1. Of note, it has been recently reported that irreversible
inhibition of g-glutamylcysteine synthetase (g-GCS), the
rate-limiting enzyme in the biosynthesis of glutathione
(GSH), an antioxidant thiol, was associated with the aug-
mentation of a pro-inflammatory signal in a ROS-sensitive
manner despite the observation that the InB-a/NF-nB sig-
naling pathway was down-regulated [32,38,40,67]. The
intriguing ability of g-GCS inhibition to block the trans-
location/activation of NF-nB and up-regulate the presum-
ably downstream cytokine pathway remains of particular
interest. It was reported that L-buthionine-(S,R)-sulfoximine
(BSO), an inhibitor of g-GCS, suppressed the oxyexcitation
(DpO2)-dependent nuclear localization of RelA (p65), the
major transactivating member of the Rel family, and sub-
sequently suppressed NF-nB activation [32,38,67]. How-
ever, in additional studies, BSO was also shown to be
capable of inducing intracellular accumulation of ROS,
particularly OH [6,7,28,29,38,83]. Taken together, these
data argue for ROS as potential second messengers for
cytokine biosynthesis; however, ROS might not be favor-
ably universal messengers in the activation of NF-nB.Furthermore, the ability of BSO to inhibit the phosphoryla-
tion/degradation of InB-a and up-regulate cytokine produc-
tion demonstrated that this transcription factor could be
partially involved, but not exclusively required, in regulat-
Fig. 7. Schematic diagram of NF-nB activation circuits and oxygen-signaling mechanisms. GSSG reduction to GSH, which is blocked by BCNU, leads to
increasing intracellular stores of [GSSG], a potent inhibitor of NF-nB transcription factor DNA binding. The pathway leading to the formation of GSH by the
action of g-GCS is blocked by BSO, inducing an irreversible inhibition of NF-nB activation. ROS are key components of the pathways leading to the activation
of NF-nB, whose binding activity is obliterated by NAC and PDTC, potent scavengers of ROS. Although NAC is elevating [GSH], it is unknown whether this
mechanism induces NF-nB activation independently from the antioxidant effects of this inhibitor. PDTC elevates GSSG concentration by GSH oxidation, a
pro-oxidant effect characteristic of dithiocarbamates, thereby mediating NF-nB inhibition. Upon NF-nB DNA binding, cascades of hyperoxia-responsive genes
are activated, which have the potential to modulate cellular response to oxidative injury.
J.J. Haddad / Cellular Signalling 14 (2002) 879–897 885
ing oxidant-mediated pathways governing pro-inflammatory
cytokines. Although a NF-nB consensus binding site is
present in the promoter region of IL-1h, IL-6, IL-8 and
TNF-a genes, among other inflammatory targets, it cannot
be positively concluded whether these specific nB moieties
are indispensable for regulating cytokine expression and
release apart from coupling this mechanism to intracellular
redox-oxidant state, and whether other transcription factors
such as AP-1 and Oct-1 are likely to be involved. However,
there is apparently dissociation between ROS-dependent
and independent pathways governing the translocation/acti-
vation of NF-nB and that oxidative signaling tightly regu-
lates this pathway, along with the downstream pro-
inflammatory cytokine route. This is rather supported by
unequivocal evidence indicating a separation of oxidant-
initiated and redox-regulated mechanisms in the NF-nBsignal transduction pathway. Therefore, the InB-a/NF-nBpathway could be partially dissociated from that of redox-
dependent regulation of pro-inflammatory cytokines, in-
dicating that this transcription factor is not exclusively
ROS-sensitive and differentially implicated in regulating
pro-inflammatory cytokine signaling. This suggests the
involvement of a possible cross-talk among several pathways
working independently or in coherence to integrate ROS
signaling mechanisms governing the regulation of inflam-
mation. In support of this view, further studies showed that
the overall NF-nB signal transduction cascade begins with a
parallel series of stimuli-specific pathways through which
cytokines (such as TNF-a and IL-1h), oxidants (such as
H2O2 and mitomycin C), and phorbol ester (such as phorbol
12-myristate 13-acetate; PMA) individually and independ-
ently can initiate signaling. These initial pathways culminate
in a common pathway through which all of the stimulating
agents ultimately signal NF-nB activation [74]. The authors
distinguished the stimuli-specific pathways by showing that
the oxidative stimuli trigger NF-nB activation in only one of
two human T-cell lines (Wurzburg but not Jurkat), whereas
TNF-a and PMA readily stimulate in both lines. The
common pathway was proposed as the simplest way of
accounting for the common requirements and properties of
the signaling pathway. A redox-regulatory mechanism in this
common pathway was also included to account for the
previously demonstrated redox regulation of NF-nB activa-
tion in Jurkat cells (in which oxidants do not activate NF-
nB); the tyrosine phosphorylation cascade was subsequently
put in the common pathway by showing that kinase activity
(inhibited by herbimycin A and tyrphostin 47) is required for
NF-nB activation by all stimuli tested in both cell lines.
Since internal sites of oxidant production have been shown
to play a key role in the cytokine-stimulated activation of
NF-nB and since tyrosine kinase and phosphatase activities
are known to be altered by oxidants, these findings suggest
that intracellular redox status controls NF-nB activation by
regulating tyrosine phosphorylation event(s) within the
common step of the NF-nB signal transduction pathway
[2,46,74,159]. Another typical model is the development of a
stable aromatic acid decarboxylase expressing the Chinese
hamster ovary cell line to study the cytotoxic properties of
intracellular and extracellular dopamine and its effect on NF-
nB [120]. The relative impermeability of cells to dopamine,
but not to L-DOPA, allows the differentiation of extracellular
and intracellular dopamine cytotoxicity. In contrast to extrac-
ellular dopamine, intracellular dopamine toxicity was resist-
ant to antioxidant protection and did not require melanin
formation for its toxicity. Furthermore, it was demonstrated
that there was a rapid and potent activation of the stress-
inducible NF-nB by intracellular dopamine, which was also
largely insensitive to antioxidant inhibition. A distinctly
slower and less potent NF-nB activation by extracellular
dopamine was blocked by antioxidants and acetylsalicylic
acid, indicating the existence of a non-oxidative mechanism
of dopamine cytotoxicity [120].
3.3. Redox-mediated regulation of NF-jB
Cellular redox status regulates various aspects of cellular
functions such as proliferation, activation, growth inhibition
and cell death [6,12,13,48,57,60,69,88,166,178,194–198].
The term ‘oxidative stress’ indicates that the antioxidant
status of cells and tissues is altered by exposure to oxidants.
More and more evidence is accumulating that a proper
balance between oxidants and antioxidants is involved in
maintaining health and longevity, and altering this balance
may cause functional disorders and disease. Oxidative
stress plays a crucial role in a number of diseases includ-
ing neuro-degenerative diseases such as stroke, Parkinson’s
and Alzheimer’s diseases, cardiovascular and autoimmune
diseases, AIDS, as well as in ischemia reperfusion injuries.
Intracellular redox-regulating molecules and enzymes such
as glutathione, catalase, superoxide dismutase, glutathione
peroxidase and thioredoxin (TRX) maintain cellular redox
status. TRX and TRX reductase, for example, exist in all
living cells and constitute the major physiological
NADPH-dependent protein disulfide redox system. TRX
is a hydrogen donor for ribonucleotide reductase, the
essential enzyme for DNA synthesis, and has a large number
of other functions in redox regulation or defense against
oxidative stress. TRX (12 kDa) has successfully been
applied to reduction of disulfides of functional importance
in different proteins including fibrinogen, Factor X, Factor
VIII, insulin, a2-macroglobulin or IgG. TRX has been shown
to regulate the glucocorticoid receptor activity and a large
number of transcription factors like NF-nB or AP-1 [119].
Glutaredoxin (GRX), together with NADPH, glutathione
(GSH) and glutathione reductase (the glutaredoxin system),
is the other major protein disulfide oxido-reductase. Gluta-
redoxin 1 from Escherichia coli (9 kDa) or human cells (12
kDa) contains a redox-active disulfide and a binding site for
GSH. GRX is a hydrogen donor for ribonucleotide reductase;
it also operates as a general protein disulfide reductase with
specificity for GSH-mixed disulfides. Glutaredoxins have a
large number of functions overlapping with thioredoxins but
J.J. Haddad / Cellular Signalling 14 (2002) 879–897886
also unique functions related to redox regulation via gluta-
thione.
The role of redox signaling in modulating the pattern of
transcription and gene expression has been well documented
[1,2,24,52,54,162,175,199–201]. NF-nB dissociation by
kinase cascade is a primary step of NF-nB activation (Fig.
7) [112]. After dissociation from InB, NF-nB must go
through the redox regulatory pathway mediated by cellular
reducing catalysts, GSH and TRX. It is well established that
NF-nB cannot bind to the nB DNA sequence of the target
genes until it is reduced. Structural biological approaches
have shed new light on the redox regulation of NF-nB. First,in early 1995 two groups independently demonstrated the
three-dimensional structure of the NF-nB subunit p50
homodimer co-crystallized with the target DNA [150,158].
NF-nB appears to have a novel DNA-binding structure
called h-barrel, a group of h sheets stretching toward the
target DNA. There is a loop in the tip of the h-barrelstructure that intercalates with the nucleotide bases and is
considered to make a direct contact with the DNA. This
DNA-binding loop contains the cysteine 62 that acts as the
target of redox regulation by a proton donor, such as GSH
and TRX. Furthermore, another group recently solved the
3D structure of TRX molecule that is associated with the
DNA-binding loop of p50 by using NMR analysis
[68,90,172]. A boot-shaped hollow on the surface of TRX
containing the redox-active cysteines could stably recognize
the DNA-binding loop of p50 and is likely to reduce the
oxidized cysteine by donating protons in a structure-depend-
ent way. Therefore, the reduction of NF-nB is considered to
be specific [89,145,202].
NF-nB binding in vitro can be inhibited by agents that
modify free sulfhydryls [28,94,164]. For example, NF-nBbinding is eliminated after treatment with N-ethylmaleimide,
an alkylating agent, and diamide, an oxidizing agent. 2-
Mercaptoethanol can reverse the diamide effect and can act
synergistically with deoxycholate plus Nonidet P-40 in
converting inactive cytosolic NF-nB to an active DNA-
binding form [203]. It is, therefore, possible that modulation
of the redox state of NF-nB could represent a post-transla-
tional control mechanism for this factor. Furthermore, nBenhancer binding proteins isolated from the nuclei of
activated human T cells have been shown to produce two
distinct nucleoprotein complexes when incubated with the
nB element from the interleukin-2 receptor-a (IL-2Ra)
gene. These two DNA–protein complexes are composed
of at least four host proteins (p50, p55, p75, p85), each of
which shares structural similarity with the v-rel oncogene
product. Nuclear expression of these proteins is induced
with distinctly biphasic kinetics following phorbol ester
activation of T cells (p55/p75 early and p50/p85 late)
[171]. DNA–protein cross-linking studies have revealed
that the more rapidly migrating B2 complex contains both
p50 and p55 while the more slowly migrating B1 complex is
composed of p50, p55, p75, and p85. Site-directed muta-
genesis of the wild-type IL-2Ra nB enhancer (GGG-
GAATCTCCC) has revealed that the binding of p50 and
p55 (B2 complex) is particularly sensitive to alteration of
the 5Vtriplet of deoxyguanosine residues. In contrast, for-
mation of the B1 complex, reflecting the binding of p75 and
p85, critically depends upon the more 3V sequences of this
enhancer element. DNA binding by all four of these Rel-
related factors is blocked by selective chemical modification
of lysine and arginine residues, suggesting that both of
these basic amino acids are required for binding to the nBelement [171]. Similarly, covalent modification of free
sulfhydryl groups with diamide (reversible) or N-ethylma-
leimide (irreversible) results in a complete loss of DNA
binding activity. In contrast, mild oxidation with glucose
oxidase selectively inhibits p75 and p85 binding while not
blocking p50 and p55 interactions. These findings suggest
that reduced cysteine thiols play an important role in the
DNA binding activity of this family of Rel-related tran-
scription factors. A further role for redox regulation in
activation of NF-nB was suggested by the observation that
the DNA binding activity of free protein, but not preformed
DNA–protein complex, is inhibited by –SH modifying
agents but enhanced by reducing agents. Mutagenesis of
conserved cysteine residues in the p50 subunit identified
amino acid 62 as being important for DNA binding, as a
serine substitution at this position reduces DNA binding
affinity, but renders the protein insensitive to –SH modify-
ing agents [36]. DNA binding activity of the wild type
protein, but not the amino acid 62 mutant, was also
stimulated by thioredoxin while detection of disulphide
cross linked dimers in p50, but not the amino acid 62
mutant, suggests that thioredoxin stimulates DNA binding
by reduction of a disulphide bond involving cysteine 62.
The physiological relevance of these findings was supported
by the observation that co-transfection of a plasmid express-
ing human thioredoxin and an HIV LTR-driven reporter
construct resulted in an NF-nB-dependent increase in the
expression of the reporter gene [36,105,113,157,176]. Thus,
modification of p50 by thioredoxin, a gene induced by
stimulation of T-lymphocytes in parallel with NF-nB trans-
location, is a likely step in the cascade of events leading to
full NF-nB activation. In addition, the hypothesis that
cellular activation events occurring in T lymphocytes and
monocytes and mediated through translocation of the tran-
scription factor NF-nB are dependent upon the constitutive
redox status of these cells was investigated. Butylated
hydroxyanisole (BHA) was found to suppress not only
PMA- or TNF-induced, but also constitutive, HIV-enhancer
activity concomitant to an inhibition of NF-nB binding
activity in vitro [204]. This was also true for KBF (p50
homodimer) binding activity in U937 cells. Secretion of
TNF, the product of another NF-nB-dependent gene, wasabolished by BHA in PMA-stimulated U937 cells. The anti-
oxidative effect of BHAwas accompanied by an increase in
thiol, but not glutathione, content in stimulated and unsti-
mulated T cell, whereas TNF stimulation itself barely
modified the cellular thiol level. Furthermore, oxidative
J.J. Haddad / Cellular Signalling 14 (2002) 879–897 887
stress obtained by the addition of H2O2 could not by itself
induce NF-nB activation. These observations suggest that
TNF and PMA do not lead to NF-nB activation through
induction of changes in the cell redox status. Rather, TNF
and PMA can exert their effect only if cells are in an
appropriate redox status, because prior modification toward
reduction with BHA treatment prevents this activation. It
appears, therefore, that a basal redox equilibrium tending
toward oxidation is a prerequisite for full activation of
transduction pathways regulating the activity of NF-nB-dependent genes [92,204]. Furthermore, in macrophages,
NF-nB can be activated by H2O2 generated by the respira-
tory burst or added exogenously. The mechanism of H2O2
signaling may involve changes in the cellular redox state or
a redox reaction at the plasma membrane; however, the site
of H2O2 action cannot be readily ascertained because of its
membrane permeability. Ferricyanide, a non-permeable
redox active anion, activated NF-nB in the macrophage cell
line, J774A.1. In contrast with exogenous H2O2, activation
by ferricyanide did not correlate with net oxidation of
NAD(P)H or glutathione, suggesting that a trans-plasma
membrane redox reaction itself was the first signaling
process in NF-nB activation [8,155,169].
Phosphoseryl/threonyl protein phosphatase inhibitors,
okadaic acid and calyculin-A, failed to induce NF-nBnuclear translocation in several primary human cells
although a marked and rapid induction was observed in
their simian virus 40 transformed counterparts [170,205].
Inability to induce NF-nB cannot be due to a non-activat-
able system since NF-nB was strongly activated by TNF. It
is also unlikely that the differential induction was due to
differential sensitivity of primary and these inhibitors
equally inhibited transformed cells to phosphatase inhibitors
as the intracellular phosphatase activities of both cell types.
However, pretreatment with H2O2 or BSO, chemicals
known to elevate directly or indirectly the intracellular
free-radical levels, enabled okadaic acid to induce nuclear
translocation of NF-nB in primary cells. Conversely, cys-
teine, an antioxidant and precursor of the free radical
scavenger, glutathione, inhibited the induction of NF-nBby TNF in primary cells, and by okadaic acid or TNF in
transformed cells. These data, taken together, suggest that
free radical-dependent oxidation and protein phosphoryla-
tion are not independent modes of NF-nB induction, but are
both required for the release of NF-nB from InB. Further-more, the differential induction of NF-nB nuclear trans-
location by okadaic acid reflects intrinsic differences in the
intracellular oxidative/redox states. The induction of NF-nBby tumor necrosis factor in primary cells suggests that this
cytokine fulfills the requirement for oxidation, possibly by
inducing the production of free radicals [170,206]. In
support of this consensus, oxidative conditions have been
reported to potentiate the activation of NF-nB and AP-1 in
intact cells, but inhibit their DNA binding activity in vitro. It
has been shown that both the activation of NF-nB and the
inhibition of its DNA binding activity is modulated in intact
cells by the physiological oxidant glutathione disulphide
(GSSG). NF-nB activation in human T lineage cells (Molt-
4), for example, by 12-O-tetradecanoyl-phorbol 13-acetate
was inhibited by dithiothreitol and this was partly reversed
by the glutathione reductase inhibitor 1,3-bis(2-chlor-
oethyl)-1-nitrosourea (BCNU) or by H2O2, indicating that
GSSG may be required for NF-nB activation [184,207].
These effects of BCNU and H2O2 were not seen in
glutathione-depleted cells. However, NF-nB and AP-1 acti-
vation were potentiated by dithiothreitol if added to cell
cultures 1 h after the phorbol ester, indicating that a shift of
redox conditions may support optimal oxidative activation
with minimal inhibition of DNA binding. In addition, the
elevation of intracellular GSSG levels by BCNU before
stimulation suppressed the chloramphenicol acetyltransfer-
ase expression dependent on NF-nB but increased that
dependent on AP-1. This selective suppression of NF-nBwas also demonstrable by electrophoretic mobility shift
assays. In vitro, GSSG inhibited the DNA binding activity
of NF-nB more effectively than that of AP-1, while AP-1
was inhibited more effectively by oxidized thioredoxin
[50,93,100,102,146,184]. It was also demonstrated that
dihydrolipoate/a-lipoate redox couple, which is a cofactor
for mitochondrial dehydrogenases reactions, influences the
DNA binding activity of NF-nB. The elimination of dithio-
threitol in the electrophoretic mobility shift assay protocol
resulted in the inability to detect DNA binding activity of
activated NF-nB. The DNA binding activity was restored by
the addition of dihydrolipoate in the binding reaction
mixture. Inhibition of NF-nB DNA binding activity by in
vitro exposure to a sulfhydryl-oxidizing agent, diamide, was
also blocked by dihydrolipoate. In contrast, the addition of
the oxidized form, a-lipoate, inhibited the NF-nB DNA
binding activity. Coincidentally, pre-incubation of Jurkat
cells with dihydrolipoate potentiated and a-lipoate
inhibited, the okadaic acid-induced NF-nB activation as
detected by assessing its DNA binding activity [92,98,101,
102,136,149,208]. These results suggest that the redox
exchange exists between lipoate and NF-nB molecules.
Redox/ROS-mediated regulation of NF-nB is schematized
in Fig. 7.
In some unprecedented, but not uncommon, conditions,
NF-nB signaling pathways might exhibit redox-insensitive
liability. Renal tubular epithelial cells, for example, are
largely resistant to oxidant-induced injury despite their
capacity to accumulate relatively high concentrations of
potentially damaging prooxidant and thiol-depleting agents.
The hypothesis that such resistance may be attributable to a
lack or deficiency of signaling transduction pathways
through which reactive oxidants have been shown to pro-
mote the activation of NF-nB was tested. NF-nB was found
to be readily activated following exposure of cultured
normal rat kidney epithelial (NRK52E) cells to LPS. How-
ever, in contrast to findings with many other cell types, the
activation of NF-nB by LPS was not substantially altered
either by pretreatment of cells with the thiol antioxidant, N-
J.J. Haddad / Cellular Signalling 14 (2002) 879–897888
acetyl-L-cysteine (NAC), or by GSH depletion. Moreover,
reactive oxidants and oxidative stress-generating chemicals
were completely without effect with respect to NF-nBactivation in NRK52E cells, even following GSH depletion.
In contrast, LPS activation of NF-nB was substantially
attenuated by the intracellular Ca2 + chelator, Quin 2AM,
and by the Ca2 + -channel inhibitor, ruthenium red. More-
over, thapsigargin, a Ca2 + -ATPase inhibitor, promoted NF-
nB activation comparable to that observed by LPS. Addi-
tionally, staurosporine, a Ca2 + -dependent protein kinase C
inhibitor, substantially decreased LPS-mediated NF-nB acti-
vation [105,120,209]. These results demonstrate that the
LPS-inducible expression of NF-nB, in contrast to many
other cell types, is not responsive to oxidative stress and is
regulated, at least in part, by redox-insensitive modulation
of intracellular Ca2 + levels. Furthermore, heme–hemo-
pexin is used as a model for intravenous heme released in
trauma, stroke and ischemia–reperfusion to investigate the
role of transcription factors. A transient increase in cellular
protein oxidation occurs during receptor-mediated heme
transport from hemopexin, which is inhibited by the non-
permeable Cu(I) chelator, bathocuproinedisulfonate. Thus,
participation of surface redox process involving Cu(I) gen-
eration is proposed to be linked to the induction of the
protective proteins heme oxygenase-1 (HO-1) and metal-
lothionein-1 (MT-1) by heme–hemopexin. The region
(� 153 to � 42) in the proximal promoter of the mouse
MT-1 gene responds to heme– and CoPP–hemopexin in
transient transfection assays and contains metal-responsive
elements for MTF-1 and an antioxidant-responsive element
(ARE) overlapping a GC-rich E-box to which USF-1 and -2
bind. No decreases in DNA binding of the diamide-oxida-
tion sensitive USF-1 and USF-2 occur upon exposure of
cells to heme–hemopexin. MTF-1 and the ARE-binding
proteins are relatively resistant to diamide oxidation and are
induced approximately eight- and two-fold, respectively, by
heme–hemopexin. BCDS prevents the nuclear translocation
of MTF-1 and NF-nB by both heme– and CoPP–hemo-
pexin complexes, as well as MT-1 mRNA induction by
CoPP–hemopexin. Thus, copper is needed for the surface
oxidation events and yet the nuclear translocation of MTF-1
in response to hemopexin occurs via copper, probably
Cu(I)-dependent signaling cascades from the hemopexin
receptor rather than the oxidation per se. These findings
provide a basis for the highly tissue-specific expression and
function of NF-nB [70,104]. In addition, increasing evi-
dence indicates that intracellular redox-insensitive status
modulates the activity of various transcriptional factors,
including NF-nB [92,157,196,210]. Using primary pas-
sage-1 human tracheo-bronchial epithelial cell cultures and
an immortalized human bronchial epithelial cell line
(HBE1), it has been observed that TNF-a enhanced NF-
nB transcriptional activity (this observation was based on
gel mobility shift assays and IL-8 promoter–reporter gene
transfection studies). TNF-a activation coincided with the
translocation of RelA (p65) from the cytoplasm to the
nucleus. Furthermore, pretreatment with NAC or gluta-
thione inhibited TNF-a-induced activation of NF-nB tran-
scriptional activity and IL-8 promoter-mediated reporter
gene expression. In contrast, elevated TRX protein levels
in cells enhanced TNF-a-dependent NF-nB transcriptional
activity and IL-8 promoter activity. This observation was
independent of the manner in which TRX was elevated in
cells (e.g., by co-transfection with a FLAG-TRX expres-
sion clone, or by direct exposure to commercially avail-
able human TRX protein). Localization of TRX protein
by anti-TRX antibody indicated an accumulation of TRX
protein in the nucleus after TNF-a treatment. The nuclear
localization phenomenon was different from the major
cytosolic accumulation of glutathione and NAC [152].
This demonstrates that the movement of TRX into the
nucleus of airway epithelial cells occurs after an inflam-
matory stress, suggesting a compartmentalization effect of
thiol chemicals in the regulation of redox-dependent tran-
scriptional activity.
4. Oxygen radicals and redox regulation of HIF-1
signaling
The heterogeneous pO2 distribution in tissue ranging
from about 0 to 90 Torr at a constant arterial pO2 of about
100 Torr requires an oxygen-sensing system to optimize
specific organ functions. Cells located at the arterial inflow
have other metabolic properties or electrical activities than
cells located at the venous end. To meet the needs for such
different functions an oxygen sensor has to control short-
and long-term adaptation of cellular functions via regulation
of ion channel conductivity and gene expression. Oxygen is
the final acceptor of electrons in the synthesis of ATP by the
mitochondrial respiratory chain and is therefore an obliga-
tory substrate for energy transformations in most biological
systems. A reduction in the level of oxygen (hypoxia) in the
extracellular milieu severely limits the ability of cells to
perform energy-dependent functions and, if the hypoxia is
severe enough, it can lead to cell death. It is, therefore, not
surprising that elaborate mechanisms have evolved which
allow cells to detect changes in oxygen tension and protect
them against hypoxia. The long-range goal of biomedical
research is to identify the molecular and cellular mecha-
nisms by which cells detect changes in oxygen tension and
how this signal is transduced into the nuclear events
responsible for altered gene expression during hypoxia.
Altered gene expression is essential for development of a
hypoxia tolerant phenotype, which is more resistant to cell
damage or death. Gene regulation is a complex biological
process that results from molecular interactions among
nuclear protein factors (transcription factors) and DNA
control sequences. These protein–DNA interactions often
occur as the result of an extracellular stimulus that is
transmitted to the nucleus by a specific signal transduction
pathway(s). Although numerous stimuli have been identi-
J.J. Haddad / Cellular Signalling 14 (2002) 879–897 889
fied which regulate gene expression, perhaps none is more
intriguing than reduced oxygen (hypoxia). Hypoxia-induced
gene expression has been implicated in a number of
physiological processes, including erythropoiesis, carotid
body chemoreceptor function, and angiogenesis, all of
which enhance the delivery of oxygen to tissue [168].
Genes involved in mediating each of these important
processes are normally activated by long-term (hours to
days) rather than acute (seconds to minutes) episodes of
hypoxia [3,211].
4.1. Oxidative stress-mediated regulation of HIF-1
An important transcription factor that is a crucial
regulatory element in sensing hypoxic conditions and
integrating an adapted response via gene expression of
oxygen-sensitive enzymes and cofactors is the HIF-1 (Fig.
8) [3,180]. The signal transduction components which link
the availability of oxygen to the activation of these tran-
scription factors are poorly defined, but are broadly
believed to hinge on the free abundance of oxidants (i.e.,
ROS) in the cytosol. In the case of HIF-1a, for example,
post-translational stability, nuclear translocation by the aryl
hydrocarbon receptor translocator (ARNT) and consensus
DNA binding are coupled with oxygen-associated changes
in both conformation and activity of a ferroheme contain-
ing protein, believed to express peroxide generation via a
NADPH oxidase-type activity [3,45]. Hypoxic cessation of
peroxide production, for example, mediates HIF-1a stabi-
lization, nuclear translocation and gene expression. The
myriad of genes directly targeted by HIF-1a is given in
Table 2.
The stability and activity of HIF-1a, first identified as a
DNA-binding activity expressed under hypoxic conditions,
increase exponentially when pO2 is lowered. The ubiquitous
activation of HIF-1a is thus consistent with the significant
role that this transcription factor plays in coordinating
adaptive responses to hypoxia [3,45]. Low oxygen condi-
tions are known to induce alterations in gene expression
serving for the adaptation to the environmental conditions.
HIF-1 consists of two subunits: HIF-1a, which is unique to
the oxygen-response, and HIF-1h, previously known as
ARNT. Whereas ARNT is constitutively expressed, hypoxia
protects HIF-1a from proteolytic degradation in protea-
somes by so far unknown mechanisms. HIF-1, therefore,
is a heterodimeric complex consisting of a- and h-subunits.ARNT (HIF-1h) can dimerize with the aryl hydrocarbon
receptor as well as with HIF-1a, because both contain
Fig. 8. Potential oxygen sensing mechanisms and the role of the transcription factor HIF-1.
Table 2
Direct HIF-1 target genes
Glucose/Energy metabolism and cell proliferation/viability
Adenylate Kinase 3, Aldolase A, Aldolase C, Enolase 1 (ENO-1), Glucose
Transporter 1, Glucose Transporter 3, Glyceraldehyde-3-phosphate
Dehydrogenase, Hexokinase 1, Hexokinase 2, Insulin-like Growth
Factor 2 (IGF-2), IGF Binding Protein 1 (IGFBP-1), IGFBP-3, Lactate
Dehydrogenase A, Phosphoglycerate Kinase 1, Pyruvate Kinase M, p21,
Transforming Growth Factor
Erythropoiesis and iron metabolism
Ceruloplasmin, Erythropoietin (EPO), Transferrin, Transferrin Receptor
Vascular development/remodeling and vasomotor tone
Adrenergic Receptor, Adrenomedullin, Endothelin-1, Heme Oxygenase 1
(HO-1), Nitric Oxide Synthase 2, Plasminogen Activator Inhibitor 1,
Vascular Endothelial Growth Factor (VEGF), VEGF Receptor FLT-1
J.J. Haddad / Cellular Signalling 14 (2002) 879–897890
helix– loop–helix and PAS (‘Per-ARNT-Sim’) domains.
Whereas HIF-1h is constitutively expressed under normoxic
conditions, HIF-1a is rapidly degraded by the ubiquitin–
proteasome system. However, under hypoxic conditions,
HIF-1a protein stabilizes and accumulates, thus allowing
the heterodimer to translocate to the nucleus and to bind
specific promoter moieties of selective genes encoding
erythropoietin (EPO), vascular endothelial growth factor
(VEGF), glycolytic enzymes and glucose transporters
(GLUT), as well as cytokines and other inflammatory
mediators [3,45]. Adaptive responses to hypoxia, therefore,
involve the regulation of gene expression by HIF-1a, at
least in part, whose expression, stability and transcriptional
activity are reported to increase exponentially on lowering
pO2. During hypoxia, multiple systemic responses are
induced, including angiogenesis, erythropoiesis and glycol-
ysis. HIF-1a is a crucial mediator for increasing the effi-
ciency of O2 delivery through EPO and VEGF [108]. A
well-controlled process of adaptation parallels this mecha-
nism with decreased O2 availability through expression and
activation of glucose transporters and glycolytic enzymes.
EPO, for example, is responsible for increasing blood O2-
carrying capacity by stimulating erythropoiesis; VEGF is a
transcriptional regulator of vascularization and glycolytic
transporters and enzymes increase the efficiency of anaero-
bic generation of ATP, the vital biological currency. It is
expected that any reduction of tissue oxygenation in vivo
and in vitro would, therefore, provide a mechanistic stim-
ulus for a graded and adaptive response mediated by HIF-
1a. HIF-1a, therefore, may play an important role not only
in regulating the transcription of pO2-controlled genes and
energy homeostasis, but also in influencing immune
responses. However, the mechanism of cytokine-dependent
regulation of the translocation and activation of HIF-1a is
currently unknown and primitive. Cytokines act as major
participants in mediating molecular responses in physiology
and pathophysiology. There is accumulating evidence, more-
over, suggesting that the conventionally known ‘pro-inflam-
matory’ cytokines act as O2-sensitive mediators, indicating
the potential to integrate O2-linked pathways mediated by
cytokines via a ROS-dependent mechanism. Direct contact
of the respiratory epithelium, for instance, with dynamic
fluctuations in pO2 at the alveolar space blood barrier
junction during pulmonary-based ventilation is likely, there-
fore, to up-regulate the transcription, biosynthesis and mobi-
lization of cytokines. This is strengthened by the evidence
implicating the epithelium in a front-line defense strategy
activated in preparation for birth into an O2-rich environ-
ment. Furthermore, the generation of ROS might induce
pulmonary damage; however, moderate oxidative stress can
induce a signaling mechanism mediated, at least in part, by
O2-responsive cytokines. ROS, for instance, can induce pro-
inflammatory cytokine biosynthesis and this response can be
abrogated by selective antioxidants, suggesting an integral
role of endogenous ROS. As such, cytokines could form a
pivotal link in ROS-dependent pathways leading to the
activation of redox-sensitive transcription factors such as
HIF-1a, whose up-regulation determines the specificity of
cellular responses to oxidative stress.
Recent investigations have revealed a novel role for ROS
signaling in mediating a non-hypoxic effect of cytokines on
HIF-1a stabilization, nuclear translocation and activation
during normoxia. Despite the fact that HIF-1a was recog-
nized as a transcriptional activator prevailing under hypoxic
conditions, ROS signaling pathways that mediate the regu-
lation of HIF-1a have emerged only recently. Consistent
with this notion, it was reported that a non-hypoxic pathway
mediating the effect of cytokines in regulating the stabiliza-
tion, translocation and activation of HIF-1a in a ROS-
sensitive mechanism. These results suggest that hypoxia
may not be the only major player in HIF-1a regulation and
that this pathway mediated by inflammatory cytokines may
play a major role in controlling HIF-1a regulation in a non-
hypoxic environment [3,45,85,129,211]. The concept, there-
fore, has been put forward that ROS and phosphorylation/
dephosphorylation events are master regulators of HIF-1a
induction and activation; however, the underlying pathways
and potential signaling mediators likely to be implicated
have yet to be identified. Regarding the mechanism of non-
hypoxic, ROS-dependent regulation of HIF-1a, a major role
for mitochondrial ROS generated at complex III site was
reported, thereby causing the accumulation of HIF-1a pro-
tein ostensibly responsible for the initiation of gene expres-
sion. Furthermore, depletion of the mitochondrial genome
has been shown to reverse ROS-mediated induction of HIF-
1a. In addition, it has been reported that HIF-1a-dependent
transcriptional activity in the induction of VEGF expression
has defined a novel hypoxia-independent mechanism regu-
lating vascular remodeling. Further afield, recent evidence
suggested that the RNS pathway regulates the stability and
activity of HIF-1a. For instance, it was shown that the
expression of NO synthase could cause HIF-1a accumula-
tion, thus underscoring the role of NO as an intracellular
activator of this transcription factor (Fig. 9) [221].
Fig. 9. The regulation of HIF-1a in oxidative stress, particularly involving a
crucial role for NO is observed.
J.J. Haddad / Cellular Signalling 14 (2002) 879–897 891
The molecular pathways defined by cytokines that poten-
tially mediate HIF-1a regulation, are not well understood.
Recently, for instance, a novel role for IL-1h and TNF-a as
regulatory mediators in stimulating the DNA-binding activ-
ity of HIF-1a has been reported, indicative of the conclusion
that this transcription factor is likely to be involved in
modulating gene expression during inflammation [85,129].
The augmented activity of HIF-1a due to IL-1h was sub-
sequently attributed, at least in part, to increased HIF-1a
protein abundance under non-hypoxic conditions, whereas
the effect of TNF-awas thought to be due to the concomitant
activation of certain proteins that were proposed to be part of
the activated complex. Moreover, cAMP-responsive element
binding protein (CREB) has been implicated in augmenting
HIF-1a activity within its site in the EPO gene enhancer.
Although no effect of cytokines on cAMP levels and protein
kinase A (PKA) activity was presented, it has been reported
that cAMP analogues prevented the in vitro suppression of
EPO production mediated by cytokines [3,45,222]. Amongst
pro-inflammatory cytokines, TNF-a and IL-1h have perhaps
been most exhaustively investigated. For example, IL-1h,like TNF-a, exerts its pleiotropic activities through ligand-
induced cross-linking of specific receptors [167]. During
inflammation, cytokines, including TNF-a and IL-1h, tran-siently activate neutrophils and macrophages, thereby caus-
ing enhanced production of O2� possibly via the activation of
NADPH oxidase. This oxidative burst involves a rapid but
transient release of ROS as a crucial part of the defense
mechanisms against invading microbial pathogens and tumor
cell metastasis. Although TNF-a and IL-1h are primarily
produced by macrophages, accumulating evidence suggests
that other cell types such as endothelial and epithelial cells
release IL-1h, IL-6, TNF-a and other inflammatory media-
tors, thereby amplifying the inflammatory responses by
activating and recruiting inflammatory cells. In this respect,
it has been reported that cytokines up-regulate intracellular
accumulation of ROS. More recently, well-defined studies
indicated that cytokines increase mitochondrial ROS gener-
ation, suggesting that their effect could be mediated through a
ROS-sensitive mechanism [3,45]. The results reported by
Haddad and Land [85,129] indicate a potential role for
cytokines in inducing the accumulation of intracellular
ROS, thereby reinforcing the notion that these mediators
exert their effect on transcription factors including HIF-1a
through a ROS-dependent mechanism. Regarding the likely
source of ROS production engendered by cytokines, at least
two sources may be involved: (i) the membrane-bound
NADPH oxidase and (ii) the mitochondrial respiratory chain.
Although ROS, in general, may be involved in mediating the
effect of cytokines on HIF-1a induction, the latter mecha-
nism probably predominates because blockade of mitochon-
drial respiration abrogates cytokine-dependent activation of
HIF-1a. Furthermore, evidence is provided that different
ROS species (O2� , OH and H2O2) may mediate the effect of
cytokines on HIF-1a stabilization, localization and acti-
vation. The observation that a non-hypoxic pathway medi-
ates the effect on HIF-1a which involves ROS generated
within the mitochondrial complex is supported by unequiv-
ocal evidence since diphenylene iodonium (DPI), an inhib-
itor of complex I nicotinamide adenine dinucleotide
phosphate-dependent oxidase (which blockades the conver-
sion of ubiquinone! ubiquinol), abrogates cytokine-medi-
ated activation of HIF-1a, indicating a crucial role for
mitochondria-derived ROS in HIF-1a signaling. Although
it has been suggested that ROS mediate their signaling by
affecting kinases and/or phosphatase activities, the precise
downstream pathway(s) affected by ROS, which govern HIF-
1a translocation/activation, have yet to be identified. It is
concluded, therefore, that the production of ROS is clearly
involved in cytokine-mediated normoxic regulation of HIF-
1a stabilization, translocation and activation [42,221].
In support of the aforementioned observations, Nickel
(Ni2 + ) and cobalt (Co2 + ) were reported to mimic hypoxia
and were used as a tool to study the role of oxygen sensing
and signaling cascades in the regulation of hypoxia-indu-
cible gene expression [212]. These metals can produce
oxidative stress; therefore, it was conceivable that ROS
may trigger signaling pathways resulting in the activation
of HIF-1 transcription factor and up-regulation of hypoxia-
related genes. It was found that the exposure of A549 cells
to Co2 + or Ni2 + produced oxidative stress, and although
Co2 + was a more potent producer of ROS than Ni2 + , both
metals equally increased the expression of Cap43, a hypo-
xia-regulated gene [116]. The co-administration of H2O2
with metals induced more ROS; however, this did not
further increase the expression of Cap43 mRNA. The free
radical scavenger 2-mercaptoethanol completely suppressed
ROS generation by CoCl2 and NiCl2 but did not diminish
the induced Cap43 gene expression. Ni2 + , hypoxia and
desferrioxamine as assessed in transient transfection assays,
stimulated the activity of the HIF-1 transcription factor, but
this activation was not diminished when oxidative stress
was attenuated nor was HIF-dependent transcription
enhanced by H2O2. It is concluded that ROS are produced
during the exposure of cells to metals that mimic hypoxia,
but the formation of ROS was not involved in the activation
of HIF-1-dependent genes (Fig. 10).
On the hypoxic mechanisms that regulate HIF-1, cad-
mium (Cd) has been reported as a substantial industrial and
environmental pollutant that seriously impairs erythropoi-
esis. Cd has been demonstrated to aggravate anemia by
suppressing erythropoietin gene expression in anemic
patients. As hypoxic induction of erythropoietin mRNA
depends on HIF-1, it was hypothesized that Cd suppresses
the hypoxic activation of HIF-1. In hypoxic Hep3B cells,
Cd suppressed all mRNAs of various genes, which are
known to be upregulated by HIF-1 activation under hypo-
xia, in a dose-dependent manner [213]. Cd inhibited the
hypoxia-induced activity of luciferase in 293 cells, which
were transfected with a reporter plasmid carrying a hypoxia
response element. By electrophoretic mobility gel shift
assay, Cd inhibited the DNA-binding activity of HIF-1 in
J.J. Haddad / Cellular Signalling 14 (2002) 879–897892
hypoxic Hep3B cells. Cd reduced the amount of HIF-1a
protein in hypoxia, whereas it did not affect HIF-1a mRNA
levels. Moreover, Cd inhibited HIF-1a accumulation in-
duced by cobalt and desferrioxamine. Antioxidants and a
proteasome inhibitor prevented the HIF-1a degradation
caused by Cd. The possibility that oxidative stress mediates
this action of Cd was subsequently examined. Cd did not
affect protein oxidation and reduced glutathione levels in
hypoxic cells. These results indicate that Cd triggers a redox/
proteasome-dependent degradation of HIF-1a protein,
reducing HIF-1 activity and in turn suppressing the hypoxic
induction of hypoxia-inducible genes [213]. Furthermore,
iron chelators are pluripotent neuronal anti-apoptotic agents
that have been shown to enhance metabolic recovery in
cerebral ischemia models [127]. The precise mechanism(s)
by which these agents exert their effects remains unclear.
Recent studies have demonstrated that iron chelators activate
a hypoxia signal transduction pathway in non-neuronal cells
that culminates in the stabilization of HIF-1 and increased
expression of gene products that mediate hypoxic adaptation.
Zaman et al. [127] examined the hypothesis that iron
chelators prevent oxidative stress-induced death in cortical
neuronal cultures by inducing expression of HIF-1 and its
target genes. It was reported that the structurally distinct iron
chelators desferrioxamine mesylate and mimosine prevent
apoptosis induced by glutathione depletion and oxidative
stress in embryonic cortical neuronal cultures. The protec-
tive effects of iron chelators are correlated with their ability
to enhance DNA binding of HIF-1 and activating tran-
scription factor 1 (ATF-1)/CREB to the hypoxia response
element in cortical cultures and the H19-7 hippocampal
neuronal cell line. It was shown that mRNA, protein, and/or
activity levels for genes whose expression is known to be
regulated by HIF-1, including glycolytic enzymes, p21
(waf1/cip1), and erythropoietin, are increased in cortical
neuronal cultures in response to iron chelator treatment.
Finally, it was demonstrated that cobalt chloride, which also
activates HIF-1 and ATF-1/CREB in cortical cultures, also
prevents oxidative stress-induced death in these cells. Alto-
gether, these results suggest that iron chelators exert their
neuroprotective effects, in part, by activating a signal trans-
duction pathway leading to increased expression of genes
known to compensate for hypoxic or oxidative stress. In
contrast, one hypothesis for oxygen sensing has postulated
that ROS generated at mitochondrial complex III are the
initiators of the hypoxic signal. It was found that mitochon-
drial DNA-devoid (Uj) cells have a normal response to
hypoxia, measured at the level of HIF-1a protein stabiliza-
tion, nuclear translocation, and its transcriptional activation
activity. Furthermore, overexpression of catalase, either in
the mitochondria or in the cytosol, fails to modify the
hypoxia response indicating that H2O2 is not a signaling
molecule in the hypoxic signaling cascade that culminates
with HIF-1 activation [4,214,215,222].
Fig. 10. Oxygen sensing proposed mechanisms for the regulation of gene transcription and the involvement of HIF-1 as a hypoxia-mediated transcriptional
activity (see discussion for further details). Abbreviations: AA, arachidonic acid; ARNT, aryl receptor hydrocarbon nuclear translocator; CREB, cAMP-
responsive element binding protein; CBP, CREB-binding protein; DAG, diacyl glycerol; ECF, extracellular fluid; HIF-1, hypoxia-inducible factor-1; ICF,
intracellular fluid; IP3, inositol triphosphate; MAPK, mitogen-activated protein kinase; PKC, protein kinase C; ROS, reactive oxygen species; SAPK, stress-
activated protein kinase.
J.J. Haddad / Cellular Signalling 14 (2002) 879–897 893
4.2. Redox-mediated regulation of HIF-1
Cellular redox state is closely related to hypoxia by
changes in the expression of redox-regulated genes and
the generation of ROS (Fig. 10) [216,221,222]. Direct
evidence was provided indicating that alteration of cellular
redox states by treating cells with H2O2 or dithiothreitol
impairs hypoxia signaling mechanisms and the expression
of HIF-1a protein in hypoxic cells. In addition, HIF-1
DNA-binding activity in vitro is sensitive to oxidizing
reagents diamide and H2O2 and the alkylating agent N-
ethylmaleimide. Of note, the activity of N-ethylmaleimide-
inactivated HIF-1 can be partially restored by addition of
nuclear extract from non-hypoxic cells [53]. Furthermore,
the regulation of HIF-1 activity is primarily determined by
the stability of the HIF-1a protein. Both HIF-1a and HIF-
1h mRNAs were constitutively expressed in HeLa and
Hep3B cells with no significant induction by hypoxia
[217]. However, the HIF-1a protein was barely detectable
in normoxic cells, even when HIF-1a was over-expressed,
but was highly induced in hypoxic cells, whereas HIF-1hprotein levels remained constant, regardless of pO2. Hypo-
xia-induced HIF-1 DNA-binding as well as the HIF-1a
protein were rapidly and drastically decreased in vivo
following an abrupt increase to normal oxygen tension.
Moreover, short pre-exposure of cells to H2O2 selectively
prevented hypoxia-induced HIF-1 binding via blocking
accumulation of HIF-1a protein, whereas treatment of
hypoxic cell extracts with H2O2 had no effect on HIF-1
binding [217,222]. These observations suggest that an intact
redox-dependent signaling pathway is required for destabi-
lization of the HIF-1a protein. In hypoxic cell extracts, HIF-
1 DNA binding was reversibly abolished by sulfhydryl
oxidation. Furthermore, the addition of reduced thioredoxin
to cell extracts enhanced HIF-1 DNA binding. Consistent
with these results, overexpression of thioredoxin and Ref-1
significantly potentiated hypoxia-induced expression of a
reporter construct containing the wild-type HIF-1 binding
site, indicating that the activation of HIF-1 involves redox-
dependent stabilization of HIF-1a protein [80,218,221,222].
HIF-a protein is continuously synthesized, but is rapidly
degraded by the ubiquitin–proteasome system under oxic
conditions. Hypoxia, transition metals, iron chelators and
several antioxidants stabilize the HIF-a proteins, allowing
the formation of the transcriptionally active HIF complex.
However, the sequences and mechanisms involved in the
regulated degradation of the a protein subunits are poorly
understood. Analysis of the available cloned sequences of
human and mouse members of the HIF-a family of proteins
revealed an area of about 15 amino acids with strong
sequence conservation between all the members [219–
221]. This area corresponds to the region encompassing
amino acids 557–571 of the hHIF-1a subunit. Fragments of
HIF-1a and HIF-3a proteins containing this conserved
sequence were able to confer hypoxia regulation when
expressed as fusion proteins in Hep3B cells. Regulation
was observed with all the known hypoxia ‘‘mimics,’’ includ-
ing the reducing thiol donor N-mercaptopropionylglycine.
Furthermore, selective alanine substitutions of amino acids
561–568 stabilized the protein in normoxic conditions. In
addition, transfection with an expression vector containing a
fragment of hHIF-1a comprising amino acids 540–580
enhanced transactivation activity of the full-length hHIF-
1a protein. These results suggest that the above-mentioned
conserved sequences are likely to be involved in the hypoxic
stabilization of HIF-a proteins. The mechanisms and the
interacting ubiquitin-ligases involved in the selective degra-
dation process, however, remain unknown. HIF-1a and HLF
are two highly related basic helix–loop–helix/Per-ARNT-
Sim (bHLH/PAS) homology transcription factors. Despite
strong similarities in their activation mechanisms (e.g., they
both undergo rapid hypoxia-induced protein stabilization,
bind identical target DNA sequences, and induce synthetic
reporter genes to similar degrees), they are both essential for
embryo survival via distinct functions during vascularization
(HIF-1a) or catecholamine production (HLF). It is currently
unknown how such specificity of action is achieved. In this
respect, it was reported here that DNA binding by HLF, but
not by HIF-1a, is dependent upon reducing redox condi-
tions. In vitro DNA binding and mammalian two-hybrid
assays showed that a unique cysteine in the DNA-binding
basic region of HLF is a target for the reducing activity of
redox factor Ref-1 [220–222]. Although the N-terminal
DNA-binding domain of HIF-1a can function in the absence
of Ref-1, it was found that the C-terminal region containing
the transactivation domain requires Ref-1 for full activity.
These data reveal that the hypoxia-inducible factors are
subject to complex redox control mechanisms that can target
discrete regions of the proteins, thereby establishing a dis-
criminating control mechanism for differential regulation of
HIF-1a and HLF activity.
5. Conclusion and future prospects
The study of gene expression and gene regulation is
critical in the development of novel gene therapies. Reac-
tive oxygen and nitrogen species (oxidative stress) are
produced in health and disease. The antioxidant defense
system—a complex system that includes intracellular
enzymes, non-enzymatic scavengers, and dietary compo-
nents—normally controls the production of ROS. Oxida-
tive stress occurs when there is a marked imbalance
between the production and removal of reactive oxygen
and nitrogen species. This imbalance arises when antiox-
idant defenses are depleted or free radicals are overpro-
duced. A growing body of evidence also exists showing
that enhancement of the oxidative stress antioxidant
defense system can reduce markers of oxidative stress.
Recognition of reactive species and redox-mediated protein
modifications as potential signals may open up a new field
of cell regulation via specific and targeted genetic control
J.J. Haddad / Cellular Signalling 14 (2002) 879–897894
of transcription factors and thus can provide us with a
novel way of controlling disease processes.
Acknowledgements
The author’s own publications are financially supported
by the Anonymous Trust (Scotland), the National Institute
for Biological Standards and Control (England), the
National Institutes of Health (NIH; USA), the Tenovus
Trust (Scotland), the UK Medical Research Council (MRC,
London) and the Wellcome Trust (London). Dr. John J.
Haddad holds the George John Livanos prize (London) and
the NIH (California, USA) award fellowship.
References
[1] Alder V, Yin Z, Tew KD, Ronai Z. Oncogene 1999;18:6104–11.
[2] Arrigo AP. Free Radic Biol Med 1993;27:936–44.
[3] Bunn HF, Poyton RO. Physiol Rev 1996;76:839–85.
[4] Caro J. High Alt Med Biol 2001;2:145–54.
[5] D’Angio CT, Finkelstein JN. Mol Genet Metab 2000;71:371–80.
[6] Haddad JJ, Land SC. Am J Physiol, Lung Cell Mol Physiol 2000;
278:L492–503.
[7] Haddad JJ, Safieh-Garabedian B, Saade NE, Kanaan SA, Land SC.
Cytokine 2001;13:138–47.
[8] Lakshminarayanan V, Drab-Weiss EA, Roebuck KA. J Biol Chem
1998;273:32670–8.
[9] Liu TZ, Lee KT, Chern CL, Cheng JT, Stern A, Tsai LY. Ann Clin
Lab Sci 2001;31:383–90.
[10] MacNeeW,Rahman I. Am JRespir Crit CareMed 1999;160:S58–65.
[11] MacNee W, Rahman I. Trends Mol Med 2001;7:55–62.
[12] Rahman I, MacNee W. Eur Respir J 2000;16:534–54.
[13] Rahman I, Mulier B, Gilmour PS, Watchorn T, Donaldson K, Jeffery
PK, et al. Biochem Pharmacol 2001;62:787–94.
[14] Remacle J, Raes M, Toussaint O, Renard P, Rao G. Mutat Res
1995;316:103–22.
[15] Schreck R, Baeuerle PA. Methods Enzymol 1994;234:151–63.
[16] Schulze-Osthoff K, Bauer MK, Vogt M, Wesselborg S. Int J Vitam
Nutr Res 1997;67:336–42.
[17] Sen CK. Biochem Pharmacol 1998;55:1747–58.
[18] Yoshida Y, Maruyama M, Fujita T, Arai N, Hayashi R, Araya J, et al.
Am J Physiol, Lung Cell Mol Physiol 1999;276:L900–8.
[19] Accaoui MJ, Enoiu M, Mergny M, Masson C, Dominici S, Wellman
M, et al. Biochem Biophys Res Commun 2000;276:1062–7.
[20] Aruoma OI, Halliwell B, Hoey BM, Beutler J. Free Radic Biol Med
1989;6:593–7.
[21] Baines DL, Ramminger SJ, Collett A, Haddad JJ, Best OG, Land
SC, et al. J Physiol 2001;532:105–13.
[22] Bernard GR. Am J Med 1991;91(3C):54S–9S.
[23] Bunn HF, Gu J, Huang LE, Park JW, Zhu H. J Exp Biol 1998;
201:1197–201.
[24] Cimino F, Esposito F, Ammendola R, Russo T. Curr Top Cell Regul
1997;35:123–48.
[25] Clemens JA. Free Radic Biol Med 2000;28:1526–31.
[26] Droge W, Schulze-Osthoff K, Mihm S, Galter D, Schenk H, Eckm
HP, et al. FASEB J 1994;8:1131–8.
[27] Gon Y, Hashimoto S, Nakayama T, Matsumoto K, Koura T, Take-
shita I, et al. Respiration 2000;5:309–13.
[28] Haddad JJ, Olver RE, Land SC. J Biol Chem 2000;275:21130–9.
[29] Haddad JJ, Safieh-Garabedian B, Saade NE, Land SC. J Pharmacol
Exp Ther 2001;296:996–1005.
[30] Haddad JJ. Am J Respir Crit Care Med (In press).
[31] Haddad JJ. Cell Signal 2002;14:799–810.
[32] Haddad JJ, Land SC. Antioxid Redox Signal 2002;4:179–93.
[33] Hayes JD, McLellan LI. Free Radic Res 1999;31:273–300.
[34] Hayes JD, McMahon M. Cancer Lett 2001;174:103–13.
[35] Ho E, Quan N, Tsai YH, Lai W, Bray TM. Exp Biol Med (May-
wood) 2001;226:103–11.
[36] Matthews JR, Wakasugi N, Virelizier JL, Yodoi J, Hay RT. Nucleic
Acids Res 1992;20:3821–30.
[37] Merker MP, Pitt BR, Choi AM, Hassoun PM, Dawson CA, Fisher
AB. Am J Physiol, Lung Cell Mol Physiol 2000;279:L413–7.
[38] Haddad JJ. Cytokines Cell Mol Ther 2000;6:177–87.
[39] Haddad JJ, Land SC. Biochem Biophys Res Commun 2000;271:
257–67.
[40] Haddad JJ. Eur Cytokine Netw 2001;12:614–24.
[41] Haddad JJ. Curr Opin Invest Drugs 2001;2:1070–6.
[42] Pugh CW, Gleadle J, Maxwell PH. Breast Cancer Res 2001;3:313–7.
[43] Rahman I, Bel A, Mulier B, Lawson MF, Harrison DJ, MacNee W,
et al. Biochem Biophys Res Commun 1996;229:832–7.
[44] Rahman I, MacNee W. Thorax 1998;53:601–12.
[45] Ratcliffe PJ, O’Rourke JF, Maxwell PH, Pugh CW. J Exp Biol 1998;
201:1153–62.
[46] Rokutan K, Teshima S, Miyoshi M, Kawai T, Nikawa T, Kishi K.
J Gastroenterol 1998;33:646–55.
[47] Roum JH, Behld R, McElvancy NG, Borok Z, Crystal RG. J Appl
Physiol 1993;75:2419–24.
[48] Sen CK. Mol Cell Biochem 1999;16:31–42.
[49] Sen R, Baltimore D. Cell 1986;46:705–16.
[50] Sen CK, Packer L. FASEB J 1996;10:709–20.
[51] Sherratt PJ, Williams S, Foster J, Kernohan N, Green T, Hayes JD.
Toxicol Appl Pharmacol 2002;179:89–97.
[52] Sun Y, Oberley LW. Free Radic Biol Med 1996;21:335–48.
[53] Wang GL, Jiang BH, Semenza GL. Biochem Biophys Res Commun
1995;212:550–6.
[54] Zwacka RM, Zhou W, Zhang Y, Darby CJ, Dudus L, Halldorson J,
et al. Nat Med 1998;4:698–704.
[55] Bowie A, O’Neill LA. Biochem Pharmacol 2000;59:13–23.
[56] Chandel NS, McClintock DS, Feliciano CE, Wood TM, Melendez
AM, Rodriguez AM, et al. J Biol Chem 2000;275:25130–8.
[57] Christman JW, Blackwell TS, Juurlink BH. Brain Pathol 2000;
10:153–62.
[58] Crapo JD, Harmsen AG, Sherman MP, Musson RA. Am J Respir
Crit Care Med 2000;162:1983–6.
[59] Gilmour PS, Brown DM, Beswick PH, MacNee W, Rahman I, Do-
naldson K. Environ Health Perspect 1997;105:1313–7.
[60] Gius D, Botero A, Shah S, Curry HA. Toxicol Lett 1999;106:
93–106.
[61] Gouze JN, Bianchi A, Becuwe P, Dauca M, Netter P, Magdalou J,
et al. FEBS Lett 2002;510:166–70.
[62] Haddad JJ, Choudhary KK, Land SC. Biochem Biophys Res Com-
mun 2001;281:311–6.
[63] Haddad JJ, Lauterbach R, Saade NE, Safieh-Garabedian B, Land SC.
Biochem J 2001;355:29–38.
[64] Haddad JJ, Collett A, Land SC, Olver RE, Wilson SM. Biochem
Biophys Res Commun 2001;281:987–92.
[65] Haddad JJ, Land SC. Am J Respir Cell Mol Biol 2002;26:114–26.
[66] Haddad JJ, Land SC. Br J Pharmacol 2002;135:520–36.
[67] Haddad JJ, Saade NE, Safieh-Garabedian B. Cell Signal 2002;14:
211–8.
[68] Hayashi T, Ueno Y, Okamoto T. J Biol Chem 1993;268:11380–8.
[69] Hudson VM. Free Radic Biol Med 2001;30:1440–61.
[70] Janssen YM, Sen CK. Methods Enzymol 1999;300:363–74.
[71] MannaSK, Tien-KuoM,Aggarwal BB.Oncogene 1999;18:4371–82.
[72] Maziere C, Conte MA, Degonville J, Ali D, Maziere JC. Biochem
Biophys Res Commun 1999;265:116–22.
[73] Nie Z, Mei Y, Ford M, Rybak L, Marcuzzi A, Ren H, et al. Mol
Pharmacol 1998;53:663–9.
J.J. Haddad / Cellular Signalling 14 (2002) 879–897 895
[74] Anderson MT, Staal FJ, Gilter C, Herzenberg LA. Proc Natl Acad
Sci U S A 1994;91:11527–31.
[75] Andrew AS, Klei LR, Barchowsky A. Am J Physiol, Lung Cell Mol
Physiol 2001;281:L607–15.
[76] Blackwell TS, Christman JW, Hagan T, Price P, Edens T, Morris PE,
et al. Antioxid Redox Signal 2000;2:93–102.
[77] Chandel NS, Trzyna WC, McClintock DS, Schumacker PT. J Im-
munol 2000;165:1013–21.
[78] Chandel NS, Schumacker PT, Arch RH. J Biol Chem 2001;276:
42728–36.
[79] Coe JP, Rahman I, Sphyris N, Clarke AR, Harrison DJ. Free Radic
Biol Med 2002;32:187–96.
[80] Ema M, Hirota K, Mimura J, Abe H, Yodoi J, Sogawa K, et al.
EMBO J 1999;18:1905–14.
[81] Garcia-Ruiz C, Colell A, Morales A, Kaplowitz N, Fernandez-Checa
JC. Mol Pharmacol 1995;48:825–34.
[82] Haddad JJ, Land SC. Biochem Biophys Res Commun 2001;285:
267–72.
[83] Haddad JJ, Safieh-Garabedian B, Saade NE, Land SC. Br J Pharma-
col 2001;133:49–60.
[84] Haddad JJ. Cytokine 2002;17:301–10.
[85] Haddad JJ. Eur Cytokine Netw 2002;13:250–60.
[86] Haddad JJ, Fahlman CS. Biochem Biophys Res Commun 2002;291:
1045–51.
[87] Haddad JJ, Land SC, Tarnow-Mordi WO, Zembala M, Kowalczyk
R, Lauterbach R. J Pharmacol Exp Ther 2002;300:567–76.
[88] Hirota K, Murata M, Sachi Y, Nakamura H, Takeuchi J, Mori K,
et al. J Biol Chem 1999;274:27891–7.
[89] Hirota K, Murata M, Itoh T, Yodoi J, Fukuda K. FEBS Lett
2001;489:134–8.
[90] Jin DY, Chae HZ, Rhee SG, Jeang KT. J Biol Chem 1997;272:
30952–61.
[91] Lee JI, Burckart GJ. J Clin Pharmacol 1998;38:981–93.
[92] Matthews JR, Hay RT. Int J Biochem Cell Biol 1995;27:865–79.
[93] Meyer M, Pahl HL, Baeuerle PA. Chem Biol Interact 1994;91:
91–100.
[94] Rahman I. Biochem Pharmacol 2000;60:1041–9.
[95] Rahman I, MacNee W. Free Radic Biol Med 2000;28:1405–20.
[96] Ravati A, Ahlemeyer B, Becker A, Klumpp S, Krieglstein J. J Neu-
rochem 2001;78:909–19.
[97] Schindl M, Oberhuber G, Pichlbauer EG, Obermair A, Birner P,
Kelley MR. Int J Oncol 2001;19:799–802.
[98] Schulze-Osthoff K, Los M, Baeuerle PA. Biochem Pharmacol 1995;
50:735–41.
[99] Song C, Al-Mehdi AB, Fisher AB. Am J Physiol, Lung Cell Mol
Physiol 2001;281:L993–1000.
[100] Staal FJ, Anderson MT, Herzenberg LA. Methods Enzymol 1995;
252:168–74.
[101] Suzuki YJ, Packer L. Methods Enzymol 1995;252:175–80.
[102] Suzuki YJ, Mizuno M, Tritschler HJ, Packer L. Biochem Mol Biol
Int 1995;36:241–6.
[103] Thompson AB, Robbins RA, Romberger DJ. Eur Respir J 1985;
8:127–49.
[104] Vanacore RM, Eskew JD, Morales PJ, Sung L, Smith A. Antioxid
Redox Signal 2000;2:739–52.
[105] Westendorp MO, Shatrov VA, Schulze-Osthoff K, Frank R, Kraft M,
Los M, et al. EMBO J 1995;14:546–54.
[106] Bunnell E, Pacht ER. Am Rev Respir Dis 1993;148:1174–8.
[107] Cantin AM, Hubbard RC, Crystal RG. Am Rev Respir Dis 1989;
139:370–2.
[108] Duyndam MC, Hulscher TM, Fontijn D, Pinedo HM, Boven E. J
Biol Chem 2001;276:48066–76.
[109] Jimenez LA, Drost EM, Gilmour PS, Rahman I, Antonicelli F,
Ritchie H, et al. Am J Physiol, Lung Cell Mol Physiol 2002;282:
L237–48.
[110] Jowsey IR, Thomson AM, Flanagan JU, Murdock PR, Moore GB,
Meyer DJ, et al. Biochem J 2001;359:507–16.
[111] Morrison D, Rahman I, Lannan S, MacNee W. Am J Respir Crit Care
Med 1999;159:473–9.
[112] Okamoto T, Sakurada S, Yang JP, Merin JP. Curr Top Cell Regul
1997;35:149–61.
[113] Piret B, Legrand-Poels S, Sappey C, Piette J. Eur J Biochem 1995;
228:447–55.
[114] Rahman I, MacNee W. Am J Physiol 1999;277:L1067–88.
[115] Rahman I, van Schadewijk AA, Hiemstra PS, Stolk J, van Krieken
JH, MacNee W, et al. Free Radic Biol Med 2000;28:920–5.
[116] Salnikow K, Su W, Blagosklonny MV, Costa M. Cancer Res 2000;
60:3375–8.
[117] Saugstad OD. Acta Pediatr 1997;86:1277–82.
[118] Tacchini L, Fusar-Poli D, Bernelli-Zazzera A. Biochem Pharmacol
2002;63:139–48.
[119] Tanaka T, Nakamura H, Nishiyama A, Hosoi F, Masutani H, Wada
H, et al. Free Radic Res 2001;33:851–5.
[120] Weingarten P, Bermak J, ZhouQY. J Neurochem 2001;76:1794–804.
[121] Brennan P, O’Neill LA. Biochem Soc Trans 1996;24:3S.
[122] Pena LR, Hill BB, McClain CJ. J Parenter Enteral Nutr 1999;23:
1–6.
[123] Rahman I, Bel A, Mulier B, Donaldson K, MacNee W. Am J Physiol
1998;275:L80–6.
[124] Rahman I. Antioxid Redox Signal 1999;1:425–47.
[125] Rahman I, Antonicelli F, MacNee W. J Biol Chem 1999;274:
5088–96.
[126] Schoonbroodt S, Piette J. Biochem Pharmacol 2000;60:1075–83.
[127] Zaman K, Ryu H, Hall D, O’Donovan K, Lin KI, Miller MP, et al.
J Neurosci 1999;19:9821–30.
[128] Barrett EG, Johnston C, Oberdorster G, Finkelstein JN. Toxicol Appl
Pharmacol 1999;158:211–20.
[129] Haddad JJ, Land SC. FEBS Lett 2001;505:269–74.
[130] Haddad JJ, Land SC, Saade NE, Safieh-Garabedian B. Biochem
Biophys Res Commun 2000;274:500–5.
[131] Haddad JJ. Biochem Pharmacol 2002;63:305–20.
[132] Haddad JJ, Land SC, Tarnow-Mordi WO, Zembala M, Kowalczyk
D, Lauterbach R. J Pharmacol Exp Ther 2002;300:559–66.
[133] Ho E, Chen G, Bray TM. Free Radic Biol Med 2000;28:604–14.
[134] Ho E, Bray TM. Proc Soc Exp Biol Med 1999;222:205–13.
[135] Jeannin P, Delneste Y, Lecoanet-Henchoz S, Gauchat JF, Life P,
Holmes D, et al. J Exp Med 1995;182:1785–92.
[136] Packer L, Roy S, Sen CK. Adv Pharmacol 1997;38:79–101.
[137] Suzuki YJ, Aggarwal BB, Packer L. Biochem Biophys Res Commun
1992;189:1709–15.
[138] Tsuji F, Miyake Y, Aono H, Kawashima Y, Mita S. Clin Exp Im-
munol 1999;115:26–31.
[139] Agani FH, Pichiule P, Chavez JC, LaManna JC. J Biol Chem 2000;
275:35863–7.
[140] Takeuchi J, Hirota K, Itoh T, Shinkura R, Kitada K, Yodoi J, et al.
Antioxid Redox Signal 2000;2:83–92.
[141] Beg AA, Finco TS, Mantermet PV, Baldwin AS. Mol Cell Biol
1993;13:3301–10.
[142] Brennan P, O’Neill LA. Biochem J 1996;320:975–81.
[143] Carter AB, Knudtson KL, Monick MM, Hunninghake GW. J Biol
Chem 1999;274:30858–63.
[144] Chae H, Chae S, Park N, Bang B, Cho S, Kim J, et al. Int Immu-
nopharmacol 2001;1:255–63.
[145] Cho S, Urata Y, Iida T, Goto S, Yamaguchi M, Sumikawa K, et al.
Biochem Biophys Res Commun 1998;253:104–8.
[146] Clive DR, Greene JJ. Cell Biochem Funct 1996;14:49–55.
[147] Deng L, Lin-Lee YC, Claret FX, Kuo MT. J Biol Chem 2001;
276:413–20.
[148] Didonato JA, Hayakawa M, Rothwarf DM, Zandi E, Karin MA.
Nature 1997;388:548–54.
[149] Flohe L, Brigelius-Flohe R, Saliou C, Traber MG, Packer L. Free
Radic Biol Med 1997;22:1115–26.
[150] Ghosh G, Van Duyne G, Ghosh S, Sigler PB. Nature 1995;373:
303–10.
J.J. Haddad / Cellular Signalling 14 (2002) 879–897896
[151] Haddad JJ. Biochem Biophys Res Commun 2002;293:252–7.
[152] Harper R, Wu K, Chang MM, Yoneda K, Pan R, Reddy SP, et al. Am
J Respir Cell Mol Biol85 2001;25:178.
[153] Ho E, Chen G, Bray TM. FASEB J 1999;13:1845–54.
[154] Jimenez LA, Thompson J, Brown DA, Rahman I, Antonicelli F,
Duffin R, et al. Toxicol Appl Pharmacol 2000;166:101–10.
[155] Josse C, Legrand-Poels S, Piret B, Sluse F, Piette J. Free Radic Biol
Med 1998;25:104–12.
[156] Koay MA, Christman JW, Segal BH, Venkatakrishnan A, Blackwell
TR, Holland SM, et al. Infect Immun 2001;69:5991–6.
[157] Matthews JR, Kaszubska W, Turcatti G, Wells TN, Hay RT. Nucleic
Acids Res 1993;21:1727–34.
[158] Muller CW, Rey FA, Sodeoka M, Verdine GL, Harrison SC. Nature
1995;373:311–7.
[159] Pieper GM, Olds C, Hilton G, Lindholm PF, Adams MB, Roza AM.
Antioxid Redox Signal 2001;3:81–8.
[160] Rosenberger J, Petrovics G, Buzas B. J Neurochem 2001;79:35–44.
[161] Sanlioglu S, Williams CM, Samavati L, Butler NS, Wang G,
McCray Jr PB, et al. J Biol Chem 2001;276:30188–98.
[162] Tanaka C, Kamata H, Takeshita H, Yagisawa H, Hirata H. Biochem
Biophys Res Commun 1997;232:568–73.
[163] Ye J, Ding M, Zhang X, Rojanasakul Y, Nedospasov S, Vallyathan V,
et al. Mol Cell Biochem 1999;198:193–200.
[164] Hirota K, Matsui M, Murata M, Takashima Y, Cheng FS, Itoh T,
et al. Biochem Biophys Res Commun 2000;274:177–82.
[165] Hirotani S, Otsu K, Nishida K, Higuchi Y, Morita T, Nakayama
H, et al. Circulation 2002;105:509–15.
[166] Janssen-Heininger YM, Poynter ME, Baeuerle PA. Free Radic Biol
Med 2000;28:1317–27.
[167] Nicod LP. Thorax 1993;48:660–7.
[168] Giatromanolaki A, Koukourakis MI, Sivridis E, Turley H, Talks K,
Pezzella F, et al. Br J Cancer 2001;85:881–90.
[169] Kaul N, Choi J, Forman HJ. Free Radic Biol Med 1998;24:202–7.
[170] Menon SD, Qin S, Guy GR, Tan YH. J Biol Chem 1993;268:
26805–12.
[171] Molitor JA, Ballard DW, Greene WC. New Biol 1991;3:987–96.
[172] Qin J, Clore GM, Kennedy WMP, Huth JR, Gronenborn AM. Struc-
ture 1995;3:289–97.
[173] Huang CY, Fujimura M, Noshita N, Chang YY, Chan PH. J Cereb
Blood Flow Metab 2001;21:163–73.
[174] Janssen-Heininger YM, Macara I, Mossman BT. Am J Respir Cell
Mol Biol 1999;20:942–52.
[175] Legrand-Poels S, Zecchinon L, Piret B, Schoonbroodt S, Piette J.
Free Radic Res 1997;27:301–9.
[176] Mitomo K, Nakayama K, Fujimoto K, Sun X, Seki S, Yamamoto K.
Gene 1994;145:197–203.
[177] Shrivastava A, Aggarwal BB. Antioxid Redox Signal 1999;1:
181–91.
[178] Hutter D, Greene JJ. J Cell Physiol 2000;183:45–52.
[179] Takuma K, Lee E, Kidawara M, Mori K, Kimura Y, Baba A, et al.
Eur J Neurosci 1999;11:4204–12.
[180] Srinivas V, Zhu X, Salceda S, Nakamura R, Caro J. J Biol Chem
1998;273:18019–22.
[181] Kohler HB, Knop J, Martin M, de Bruin A, Huchzermeyer B, Leh-
mann H, et al. Vet Immunol Immunopathol 1999;71:125–42.
[182] Kretz-Remy C, Arrigo AP. Biofactors 2001;14:117–25.
[183] Schreck R, Meier B, Mannel DN, Droge W, Baeuerle PA. J Exp Med
1992;175:1181–94.
[184] Galter D, Mihm S, Droge W. Eur J Biochem 1994;221:639–48.
[185] Matsui N, Satsuki I, Morita Y, Inaizumi K, Kasajima K, Kanoh R,
et al. Jpn J Pharmacol 2000;84:363–6.
[186] Pepperl S, Dorger M, Ringel F, Kupatt C, Krombach F. Am J Phys-
iol, Lung Cell Mol Physiol 2001;280:L905–13.
[187] Kohler HB, Huchzermeyer B, Martin M, De Bruin A, Meier B, Nolte
I. Vet Dermatol 2001;12:129–37.
[188] Dumont A, Hehner SP, Hofmann TG, Ueffing M, Droge W, Schmitz
ML. Oncogene 1999;18:747–57.
[189] Li YP, Atkins CM, Sweatt JD, Reid MB. Antioxid Redox Signal
1999;1:97–104.
[190] Reimund J-M, Allison AC, Muller CD, Dumont S, Kenney JS, Bau-
mann R, et al. Eur J Clin Invest 1998;28:145–50.
[191] Rovin BH, Dickerson JA, Tan LC, Fassler J. Cytokine 1997;9:
178–86.
[192] Schoonbroodt S, Legrand-Poels S, Best-Belpomme M, Piette J. Bio-
chem J 1997;321:777–85.
[193] Ginis I, Hallenbeck JM, Liu J, Spatz M, Jaiswal R, Shohami E. Mol
Med 2000;6:1028–41.
[194] Gosset P, Wallaert B, Tonnel AB, Fourneau C. Eur Respir J 1999;14:
98–105.
[195] Griffith OW, Meister A. J Biol Chem 1979;254:7558–60.
[196] Meister A. J Biol Chem 1988;263:17205–8.
[197] Neuschwander-Tetri BA, Bellezzo JM, Britton RS, Bacon BR, Fox
ES. Biochem J 1996;320:1005–10.
[198] Parmentier M, Hirani N, Rahman I, Donaldson W, MacNee W, An-
tonicelli F. Eur Respir J 2000;16:933–9.
[199] Ginn-Pease ME, Whisler RL. Free Radic Biol Med 1998;25:
346–61.
[200] Tewes F, Bol GF, Brigelius-Flohe R. Eur J Immunol 1997;27:
3015–21.
[201] Valle-Blazquez M, Luque I, Collantes E, Aranda E, Solana R, Pena J,
et al. Immunology 1997;90:455–60.
[202] Gebel S, Muller T. Toxicol Sci 2001;59:75–81.
[203] Toledano MB, Leonard WJ. Proc Natl Acad Sci U S A 1991;88:
4328–32.
[204] Israel N, Gougerot-Pocidalo MA, Aillet F, Virelizier JL. J Immunol
1992;149:3386–93.
[205] Mahon TM, Brennan P, O’Neill LA. Biochem Soc Trans 1993;
21:389S.
[206] Kim JI, Ju WK, Choi JH, Choi E, Carp RI, Wisniewski HM, et al.
Brain Res Mol Brain Res 1999;73:17–27.
[207] Hardwick SJ, Adam A, Smith LL, Cohen GM. Biochem Pharmacol
1990;39:581–9.
[208] Chen F, Ye J, Zhang X, Rojanasakul Y, Shi X. Arch Biochem Bio-
phys 1997;338:165–72.
[209] Waris G, Huh KW, Siddiqui A. Mol Cell Biol 2001;21:7721–30.
[210] Li T, Shi MM, Forman HJ. Arch Biochem Biophys 1997;342:
126–33.
[211] Palmer LA, Gaston B, Johns RA. Mol Pharmacol 2000;58:
1197–203.
[212] Gong P, Hu B, Stewart D, Ellerbe M, Figueroa YG, Blank V, et al.
J Biol Chem 2001;276:27018–25.
[213] Chun YS, Choi E, Kim GT, Choi H, Kim CH, Lee MJ, et al. Eur J
Biochem 2000;267:4198–204.
[214] Srinivas V, Leshchinsky I, Sang N, King MP, Minchenko A, Caro J.
J Biol Chem 2001;276:21995–8.
[215] Vaux EC, Metzen E, Yeates KM, Ratcliffe PJ. Blood 2001;98:
296–302.
[216] Williams KJ, Telfer BA, Airley RE, Peters HP, Sheridan MR, van der
Kogel AJ, et al. Oncogene 2002;21:282–90.
[217] Huang LE, Arany Z, Livingston DM, Bunn HF. J Biol Chem 1996;
271:32253–9.
[218] Salceda S, Caro J. J Biol Chem 1997;272:22642–7.
[219] Srinivas V, Zhang LP, Zhu XH, Caro J. Biochem Biophys Res
Commun 1999;260:557–61.
[220] Lando D, Pongratz I, Poellinger L, Whitelaw ML. J Biol Chem 2000;
275:46118–27.
[221] Sandau KB, Fandrey J, Brune B. Blood 2001;97:1009–15.
[222] Carrero P, Okamoto K, Coumailleau P, O’Brien S, Tanaka H, Poel-
linger L. Mol Cell Biol 2000;20:402–15.
J.J. Haddad / Cellular Signalling 14 (2002) 879–897 897