methods for evaluating the potency and efficacy of antioxidants
TRANSCRIPT
Methods for evaluating the pote
ncy and efficacy of antioxidantsMickael Laguerrea, Eric A. Deckera, Jerome Lecomteb and Pierre VilleneuvebaDepartment of Food Science, University ofMassachusetts, Chenoweth Laboratory, Amherst,Massachusetts, USA and bCIRAD, UMR IATE,Montpellier, France
Correspondence to Pierre Villeneuve, CIRAD, UMRIATE, Montpellier F-34398, FranceTel: +33 04 67 61 55 18; fax: +33 04 67 61 55 15;e-mail: [email protected]
Current Opinion in Clinical Nutrition and
Metabolic Care 2010, 13:518–525
Purpose of review
The aim of this article is to present a brief panorama of the most widely used methods
and of new analytical approaches for evaluating antioxidant capacity and to discuss
them in terms of advantages and drawbacks.
Recent findings
To date, many in-vitro tests are available from the chemical assay performed in a
homogenous solution such as oxygen radical antioxidant capacity assay to more
complex cell-based methods using exogenic probes to detect oxidation. In complement
to these existing methods, novel approaches have recently been developed such as the
conjugated autoxidizable triene assay implemented in emulsions and using tung oil as
ultraviolet probe.
Summary
The complexity and diverse range of research topics investigated have led to the
development of a multitude of tests, but unfortunately none of them are universal. Thus,
one of the major challenges is to know which method is best suited for a particular
application.
Keywords
antioxidant capacity, conjugated autoxidizable triene assay, cell-based methods,
fluorescent probes, fluorogenic probes, oxygen radical absorbance capacity assay
Curr Opin Clin Nutr Metab Care 13:518–525� 2010 Wolters Kluwer Health | Lippincott Williams & Wilkins1363-1950
‘Progress in science depends on new techniques, new
discoveries, and new ideas, probably in that order.’
Sydney Brenner, 2002 Nobel Prize Winner in Physiology
and Medicine.
IntroductionFirst of all, it is important not to just consider antioxidant
capacity as being merely the reactivity of a compound to
reduce free radicals (and related reactive species) or
chelate transition metals. More importantly, the very
concept of antioxidant involves the notion of protecting
‘something’ from oxidation. But, what is that something?
Krinsky [1] has defined antioxidants as ‘compounds that
protect biological systems against the potentially harmful
effects of processes or reactions that cause extensive
oxidation’. Halliwell and Gutteridge [2] proposed that
an antioxidant is a ‘substance that, when present at low
concentrations compared to those of an oxidizable sub-
strate, significantly delays or prevents oxidation of that
substrate’. These two definitions are complementary, as
an oxidizable substrate is usually regarded as a biologi-
cally important molecule such as lipids, proteins, DNA,
and so on, whose oxidation leads to harmful effect. To
complicate matters further, many oxidation products of
antioxidants may still exhibit residual antioxidant
1363-1950 � 2010 Wolters Kluwer Health | Lippincott Williams & Wilkins
activity. In this way, a biological antioxidant could be
defined as a ‘substance that, when present at low con-
centrations compared to an oxidizable substrate, protects
(by itself and through its oxidation products) that sub-
strate from oxidation, and ultimately protects the organ-
ism from harmful effects of oxidative stress’.
Keeping this definition in mind, the question arises of
how to accurately evaluate the efficacy of antioxidants.
Many rapid in-vitro assays in test tubes or in cultured cells
are now available. The experimental models involve
various systems, from the simplest such as chemical
assays in homogeneous solution to more complex ones,
including heterogeneous systems such as emulsion, lipo-
some, or lipoprotein. Then, increasing the complexity
leads to living systems, including cells, animal models of
oxidative stress, and ultimately clinical tests in humans
(Fig. 1). The aim of this article is to present a brief
panorama of widespread methods and new analytical
approaches.
Test tube-based methodsAmong the multitude of test tube methods (Fig. 1),
we have focused on the widespread ones, especially
fluorescein-based oxygen radical absorbance capacity
DOI:10.1097/MCO.0b013e32833aff12
Methods for evaluating antioxidants Laguerre et al. 519
Figure 1 Methods classification as a function of the complexity of the system
aDPPH: 2,2-diphenyl-1-picrylhydrazyl radical. bFRAP: ferric-reducing antioxidant power. cCUPRAC: cupric reducing antioxidant capacity. dABTS: 2,20-azino-bis(3-ethylbenzthiazoline-6-sulphonic acid). eORACbPE: b-phycoerythrin-based oxygen radical absorbance capacity. fORACFL: fluorescein-basedoxygen radical absorbance capacity. gTRAP: total radical-trapping antioxidant parameter. hCAT: conjugated autoxidizable triene. iSPME-GC: solid phasemicroextraction coupled to gas chromatography. jTBA: thiobarbituric acid. k4-HNE: 4-hydroxynonenal. lIn this context, in vitromeans that the animal tissuesare collected fromanimal and thenundergooxidation in test tube,whereas in vivomeans that the animal is ‘submitted’ tooxidativestressand thensacrificedto collect tissues. In one case, the test tube is the ‘medium’ (in vitro) and in the other one, the organism is the ‘medium’ (in vivo).
Figure 2 Chemical structure of disodium salt of fluorescein
COONa
OONaO
(ORACFL) assay and lipid oxidation measurement as well
as the newly developed conjugated autoxidizable triene
(CAT) assay.
Fluorescein-based oxygen radical absorbance capacity
method
The ORACFL method using fluorescein (Fig. 2) as oxi-
dizable substrate [3] results from a modification of the
ORACb-PE method [4] using b-phycoerithrin, which also
results from the original Glazer’s method [5,6]. The
ORACFL method is based on the loss of fluorescence
emission of fluorescein (lex/em: 490/515 nm) when oxi-
dized by peroxyl radicals derived from 20,20-azobis(ami-
dinopropane) dihydrochloride (AAPH) in a phosphate
buffer (pH 7.4); this fluorescence decay being monitored
using a fluorimeter with 1-cm cuvette or using a micro-
plate reader. The presence of antioxidants results in the
reduction of some of the peroxyl radicals, rendering them
unavailable to oxidize fluorescein, what leads to a
decrease in loss of fluorescence. The information on
the fluorescence decay is extracted through the calcu-
lation of the area under the curve and expressed as Trolox
equivalent. Trolox is a water-soluble a-tocopherol deriva-
tive that acts as a useful standard in this and several
other assays.
520 Assessment of nutritional status and analytical methods
As the method allows only the assessment of water-
soluble compounds, a new protocol was implemented
to solubilize lipophilic molecules in aqueous buffer using
randomly methylated b-cyclodextrins and acetone [7].
To date, two distinct protocols exist: one dedicated to
hydrophilic antioxidants (H-ORACFL) and another to
lipophilic molecules (L-ORACFL). In the case of blood
plasma, Prior et al. [8] assumed that H-ORACFL and
L-ORACFL values can be summated to give a total value
(T-ORACFL), estimating the whole antioxidant capacity
of blood plasma. This is, however, questionable, as
lipophilic and hydrophilic antioxidants are assessed in
different test tubes. Thus, the possible synergistic (or
antagonistic) effect(s) occurring from the interaction in
the bloodstream between antioxidants of different
polarity is not taken into account. In addition, antioxidant
(0.5–5mmol/l) is tested at concentrations much in excess
to fluorescein (63 nmol/l); thus, the conditions do not
meet the antioxidant definition of Halliwell and Gutter-
idge [2]. Despite these criticisms and because it is easy-
to-use, rapid, and high-throughput, this widespread
method has been used in various purposes, mainly for
assessing plant extracts or foodstuffs [9,10,11�] and a
comprehensive database of ORAC values is now available
at ORACValues.com (�300 foods so far).
Conjugated autoxidizable triene method
In 2008, we developed a new method called CAT, using
tung oil as oxidizable substrate [12]. Triacylglycerols
(TAGs) from this commercially available oil contain
85% eleostearic acid, encompassing a conjugated triene
(Fig. 3) [13�], which exhibits a strong ultraviolet (UV)
absorption at 273 nm. In emulsion and under oxidizing
conditions, the degradation of conjugated triene TAGs is
accompanied by a bleaching at 273 nm (Fig. 4a) [12,13�].
Addition of antioxidants results in a delay of oxidative
process (Fig. 4b) and enables the quantification of the
antioxidant capacity through the area under the curve
(Fig. 4c). This method has been applied to flavonoids
[12], phenolic acids [12], chlorogenate [14�] and rosmar-
inate esters [15�] as well as olive leaf extracts [16�].
Although efforts must be brought to enhance its repro-
ducibility, the CAT method already presents several
Figure 3 Chemical structure of trieleostearin
sn1
O
C
O
(CH2)7
(
C
O
O
sn3O
sn2
CO (
For simplicity, eleostearic acid is depicted in its alpha configuration [9(c), 1
advantages. First, as the ORACFL method, it is high-
throughput being performed in 96-well microplate
reader. In addition, as it uses TAG constituting the major
lipids found in biological and food systems (with phos-
pholipids), the CAT assay could provide more relevant
results than the other tests using nonrepresentative sub-
strates such as ORACFL method. Regarding this matter,
we recently reported a surprising correlation (R2¼ 0.87)
between CAT values measured in emulsion [14�] and the
antioxidant capacity of chlorogenate esters analyzed on
reactive oxygen/nitrogen species (RONS) overexpressing
fibroblasts (Laguerre M, et al., in preparation). This study
used 20,70-dichlorodihydrofluorescein as the fluorogenic
probe to measure the modulation of the oxidative stress
in fibroblasts induced by a homologous series of chlor-
ogenate esters and showed for the first time that the
relationship between hydrophobicity and antioxidant
capacity follows a nonlinear trend already observed in
emulsion.). Indeed, both assays showed dodecyl chlor-
ogenate as the more active compound. Work is in progress
to determine whether this result is a coincidence or,
more interestingly, whether the simple CAT assay allows
gaining reliable insight into the antioxidant properties
in biological systems such as cultured cells. Finally, the
possibility to assess both hydrophilic and lipophilic com-
pounds using methanolic predissolution of antioxidants
[14�] constitutes another interesting advantage and makes
it a promising supplement to currently used methods.
Measurement of lipid oxidation in emulsions,
liposomes, lipoproteins, and animal tissues
In contrast to ORACFL and CAT method whose kinetic
approach is based on the monitoring of the substrate loss,
the measurement of oxidation, especially lipid oxidation,
can employ a reverse kinetic strategy based upon the
monitoring of the appearance of oxidation products.
Although methods based on the assessment of oxidation
product formation are very sensitive and suitable for most
cases [micelles, emulsion, liposomes, low-density lipo-
protein (LDL), and animal tissues], they nevertheless
suffer from the lack of any universal oxidation marker
and, therefore, can have limited applicability. Indeed, in
the particular case of polyunsaturated lipids, oxidation
109
CH2)7
11 13 Conjugated triene
CH2)7
1(t), 13(t)]. Reproduced with permission from [13�].
Methods for evaluating antioxidants Laguerre et al. 521
Figure 4 Evolution of the ultraviolet spectrum of a stripped tung oil-in-water emulsion
(a) Example of a three-dimensional depiction of the evolution of the ultraviolet spectrum of a stripped tung oil-in-water emulsion (pH 7.2) duringaccelerated oxidation by 2,2-azobis(2-amidinopropane) dihydrochloride (AAPH) at 378C. (b) Example of kinetics of relative absorbance bleaching at273nm in the absence and presence of various concentrations of Trolox in stripped tung oil-in-water emulsion during AAPH-mediated oxidation. Thereaction mixture contained 115mmol/l tung oil, 17mmol/l Brij 35, 1mmol/l AAPH, and 0.25–2mmol/l Trolox in phosphate-buffered saline (PBS), pH7.2, at 378C. (c) Example of the net protection area under the curve (AUC Sample – AUCBlank) versus Trolox concentration. Adapted from [12] and [13�].
leads to the formation of primary oxidation products
(hydroperoxides and conjugated dienes), which are then
oxidized to secondary oxidation products [malondialde-
hyde (MDA), 4-hydroxy-2-nonenal, hexanal] that can
react with free amino groups of phospholipids, proteins,
DNA, RNA, and so on to form tertiary oxidation products
what leads to a complex network of reactions. It is,
therefore, essential to evaluate numerous oxidation com-
pounds to obtain a reliable overall picture of oxidation
status, which is tedious.
Regarding primary oxidation products, two main meth-
odologies can be implemented depending on the chemi-
cal group that is evaluated: the hydroperoxide group
(–C–OOH) or the conjugated diene system (–C=C–
C=C–C). First, hydroperoxides can be estimated by
iodometric, thiocyanate [17–19], orange xylenol [20],
gluthatione peroxidase [21], or diphenyl-1-pyrenylpho-
sphine (DPPP) [22�] assays. Concerning conjugated
dienes, their presence in oxidized natural fats (contain-
ing polyunsaturated fats) has been known for almost
80 years [23] and can be monitored spectrophotometri-
cally at 234 nm in both classical 1-cm cuvettes and
96-well microplates.
Secondary oxidation products such as aldehydes (propa-
nal, hexanal,. . .) can be collected and quantified by
coupling an extraction procedure (solid phase microex-
traction, dynamic headspace), a separation step by gas
chromatography, and finally detection by flame ionization
detector, mass spectrometer, or more sensitive detectors.
Although this methodology is reliable because most of
the oxidation products are identified, it is, nevertheless,
both time and sample consuming and can lead to a poor
reproducibility. An alternative is the well known thio-
barbituric acid (TBA) based on the condensation of MDA
with TBA to form a chromogen (lmax: 532 nm; Fig. 5)
[13�]. This method has, however, been criticized as
MDAs are not always specific to lipid oxidation. Indeed,
it can result from the oxidation of glucides, amino acids,
DNA, ascorbate, and deoxyglucose [13�]. In addition,
TBA can react with other compounds than MDA. So,
the initial specific evaluation of MDA is progressively
substituted by the less-specific notion of ‘TBA-reactive
substances, TBARS’; these latter limitations can be over-
looked after a preliminary purification of TBA/MDA
complex by high-performance liquid chromatography
techniques [24,25]. Moreover, according to the model
by Dahle et al. [26], MDA can only result from the
oxidation of fatty acids containing at least three double
bonds. This means that comparison of influence of v-3-
rich diet (those containing three double bonds) in com-
parison to v-6-rich diet (those containing less than two
double bonds) on lipid oxidation through the TBA assay
is totally wrong [13�].
Finally, these aldehydes can further react in vitro and
in vivo with amino groups of phospholipids, proteins,
DNA, and so on leading to lipofuscins (sometimes coined
as tertiary oxidation products) that exhibit fluorescent
522 Assessment of nutritional status and analytical methods
Figure 5 Formation of the chromogen product (lmax : 532nm) between malondialdehyde and 2-thiobarbituric acid
MDA, malondialdehyde; TBA, 2-thiobarbituric acid. Reproduced with permission from [13�].
properties (lex: 340–390; lem: 430–490 nm) measurable
by fluorimetry [27].
Cell-based methodsThe aim of the cell-based method is to monitor oxidation
of a given substrate with or without antioxidants. How-
ever, in such a complex system, it is almost impossible to
distinguish the signal of any endogenous oxidizable sub-
strate from the ‘cellular background noise’. This has led
to the use of exogenous artificial probes exhibiting
specific fluorescence properties.
Incorporation of fluorescent probes
Some fluorescent oxidizable substrates whose disappear-
ance can be monitored are cis-parinaric acid (cPnA), C11-
BODIPY581/591, BODIPY665/676, and alkylamide or phos-
pholipidic derivatives of fluorescein (Fig. 6) [13�]. These
probes can be used in aqueous dispersion and in liposo-
mal systems, but they can also be incorporated into
biological particles (LDL) or into living cells (via a
metabolic pathway in this latter case). The resulting
fluorescence can be observed by microscopy or measured
by spectrofluorimetry or flow cytometry. Overall, spectro-
fluorimetry is better suited to measuring adherent cells
such as fibroblasts, whereas flow cytometry is a better
choice for determining cells growing in suspension, such
as lymphocytes.
For instance, cPnA (Fig. 6a) has been extensively used to
measure lipid peroxidation in erythrocytes [28,29], sub-
mitochondrial particles [30], sarcoplasmic reticulum cells
[31], rat aortic smooth muscle cells [32], macrophages
[33], neonatal rat cardiomyocytes [34], and rapidly divid-
ing cell lines such as human leukemia cells [35]. More
recently, it has been incorporated to mitochondria iso-
lated from renal proximal tubular cells [36], acute
myeloid leukemia cell lines [37�], and lymphocytes
[38�]. Among other advantages, cPnA is a bioanalogue,
does not disturb the lipid bilayer, and has a broad fluor-
escence Stokes shift (�100 nm). However, cPnA acid is
air sensitive, is photolabile, and dimerizes under light,
which can make it difficult to use [39].
C11-BODIPY581/591 is a fatty acid analogue (Fig. 6b)
displaying red fluorescence. Once oxidized, the fluor-
escence shifts from red (�590 nm) to green (�520 nm;
Fig. 7) [40]. This probe has been used to monitor lipid
oxidation in boar [41,42�], equine [43], and human [44,45]
spermatozoa, rat fibroblasts [46], human dermal fibro-
blasts [47], human liver carcinoma cell (HepG2) [47],
neuronal human astrocytes [47], and Jurkat cells [48��].
Note that C11-BODIPY581/591 is not as biomimetic as
cPnA, but is in turn, less prone to photobleaching [49] and
about twice as sensitive to oxidation compared to cPnA
[50]. Other BODIPY derivatives can also be used such as
BODIPY665/676 (Fig. 6c), which is more oxidizable and
presents a slightly broader fluorescence Stokes shift than
that of C11-BODIPY581/591 [51].
Regarding alkylamide (Fig. 6d) or phospholipidic
(Fig. 6e) derivatives of fluorescein, their excitation wave-
length (488 nm) seems to be especially well suited to
routine use in flow cytometry, for which a laser emitting
visible blue light (488 nm) is used. In a large cell popu-
lation, flow cytometry allows the study of lipid peroxi-
dation cell by cell [52,53], which is a useful tool. How-
ever, these fluorescent probes are not yet widely used for
this purpose.
Incorporation of fluorogenic probe
In contrast to fluorescent probes losing their fluorescence
when oxidized, fluorogenic probes exhibit fluorescence
when oxidized. The basic principle consists of monitor-
ing the level of fluorescence as an estimation of the level
of oxidizing species in cultured cells. One can cite dihy-
dro-derivatives of 20,70-dichlorofluorescein (Fig. 8), fluor-
escein, and ethidium constituting the most widely used
probes. Depending on their charge, their chemical struc-
ture, and the cells involved, these probes can move into a
specific cell compartment: mitochondrion for dihydro-
fluorescein [54], nucleus for dihydroethidium [55], and
cytoplasm for 20,70-dihydrodichlorofluorescein [55]. By
Methods for evaluating antioxidants Laguerre et al. 523
Figure 6 Chemical structures of some lipid-soluble fluorescent probes
Chemical structure of (a) cis-parinaric acid, (b) C11-BODIPY581/591, (c) BODIPY665/676, (d) alkylated derivatives of fluorescein, and (e) phospholipidicderivative of fluorescein. Reproduced with permission from [13�].
example, this latter has been recently incorporated to
RONS (reactive oxygen/nitrogen species) overexpres-
sing fibroblasts to study antioxidant capacity of chloro-
genate ester (Laguerre M et al., in preparation) and
Figure 7 Emission spectra of 0.05mol% C11-BODIPY581/591 in
250mmol/l egg-phosphatidylcholine vesicles
Oxidation was induced with 250mmol/l CumOOH/100nmol/l heminand spectra were recorded every 20min. The spectra show a decreasein fluorescence at 595nm, with a concomitant increase in fluorescenceat 520nm and a shoulder at 545nm. Insert: molecular structure of C11-BODIPY581/591. At arrows: the diene interconnection is most likely thetarget for free radical-induced oxidation. Reproduced with permissionfrom [40].
showed for the first time that increasing hydrophobicity
does not necessarily lead to a more efficient anti-
oxidant drug.
In terms of advantages, these probes, generally dissolved
in dimethylsulfoxide and stored at �808C, are easy-to-use
(as much as fluorescent probes). The major concern is the
ambiguity of the response, whether these probes detect a
general oxidative stress or apoptosis. Indeed, cytochrome
c, whose release by mitochondria in cytosol is a key event
in apoptosis [56], strongly oxidizes 20,70-dichlorodihydro-
fluorescein [57]. Regarding this matter, it has been shown
that the antiapoptotic proto-oncoprotein bcl-2 prevents
20,70-dichlorodihydrofluorescein oxidation [58], which
suggested that bcl-2 prevents apoptosis through an anti-
oxidant pathway. In contrast, Burkitt and Wardman [57]
refute any antioxidant pathway and assumed that the
prevention of 20,70-dichlorodihydrofluorescein oxidation
is an artefact resulting from an apoptotic pathway leading
to the prevention of mitochondrial cytochrome c release,
which is thus unable to oxidize the probe located in the
cytosol. The use of fluorogenic probes has also been the
focus of criticism regarding their absence of specificity
toward RONS. Indeed, it is unclear what kind of species
react with these probes and what makes the latter the
‘markers’ of a general oxidative stress rather than of a
precise oxidative pathway.
524 Assessment of nutritional status and analytical methods
Figure 8 Bi-electronic oxidation of 20,70-dichlorodihydrofluorescein to 20,70-dichlorofluorescein
Reproduced with permission from [13�].
ConclusionWe have seen that the complexity and diversity of
investigation systems have led to the development of
a broad range of tests, but unfortunately, none of them
has the universal scope we are seeking and none of them
is free of criticism. In this context, it is preferable to use
several methods to assess multifaceted antioxidants.
Ultimately, the answer to the question, ‘what is the best
antioxidant?’ is dependent on the system in which this
activity is measured, especially pro-oxidants, cellular
compartment, and conditions. For instance, vitamin E
reportedly is the most important [59] and one of the least
important [60] plasma antioxidants depending on the
different assay conditions used. In other words, a ‘good’
antioxidant in a given system can be a ‘bad’ one in
another system, which means that it clearly does not
make sense to just consider the magnitudes of the anti-
oxidant capacities as being a value universally applicable
for all media, cells, oxidation conditions, or substrates
[39].
References and recommended readingPapers of particular interest, published within the annual period of review, havebeen highlighted as:� of special interest�� of outstanding interest
Additional references related to this topic can also be found in the CurrentWorld Literature section in this issue (pp. 595–596).
1 Krinsky NI. Mechanism of action of biological antioxidants. Proc Soc Exp BiolMed 1992; 200:248.
2 Halliwell B, Gutteridge JM. Role of free radicals and catalytic metal ions inhuman disease: an overview. Methods Enzymol 1990; 186:1–85.
3 Ou B, Hampsch-Woodill M, Prior RL. Development and validation of animproved oxygen radical absorbance capacity assay using fluorescein asthe fluorescent probe. J Agric Food Chem 2001; 49:4619–4626.
4 Cao G, Alessio HM, Cutler RG. Oxygen-radical absorbance capacity assayfor antioxidants. Free Radic Biol Med 1993; 14:303–311.
5 Glazer AN. Fluorescence-based assay for reactive oxygen species: a pro-tective role for creatinine. FASEB J 1988; 2:2487–2491.
6 Glazer AN. Phycoerythrin fluorescence-based assay for reactive oxygenspecies. Methods Enzymol 1990; 186:161–168.
7 Huang D, Ou B, Hampsch-Woodill M, et al. Development and validation ofoxygen radical absorbance capacity assay for lipophilic antioxidants usingrandomly methylated b-cyclodextrin as the solubility enhancer. J Agric FoodChem 2002; 50:1815–1821.
8 Prior RL, Hoang HA, Gu L, et al. Assays for hydrophilic and lipophilicantioxidant capacity (oxygen radical absorbance capacity (ORACFL)) ofplasma and other biological and food samples. J Agric Food Chem 2003;51:3273–3279.
9 Schauss AG,Wu X, Prior RL, et al. Antioxidant capacity and other bioactivitiesof the freeze-dried Amazonian palm berry, Euterpe oleraceae Mart. (acai). JAgric Food Chem 2006; 54:8604–8610.
10 Seeram NP, Aviram M, Zhang Y, et al. Comparison of antioxidant potency ofcommonly consumed polyphenols-rich beverages in the United States. J AgricFood Chem 2008; 56:1415–1422.
11
�Chu Y-F, Brown PH, Lyle BJ, et al. Roasted coffees high in lipophilicantioxidants and chlorogenic acid lactones are more neuroprotective thangreen coffees. J Agric Food Chem 2009; 57:9801–9808.
Coffee roasting leads to a 30-fold increase in antioxidant capacity measured byL-ORACFL method and is more neuroprotective than green coffee.
12 Laguerre M, Lopez Giraldo LJ, Lecomte J, et al. Conjugated autoxidizabletriene (CAT) assay: a novel spectrophotometric method for determination ofantioxidant capacity using triacylglycerol as ultraviolet probe. Anal Biochem2008; 380:282–290.
13
�Laguerre M, Lopez Giraldo LJ, Lecomte J, Villeneuve P. Widespread methodsand new analytical approaches in antioxidant evaluation. Inform 2009;20:328–332.
This mini-review covers the different methods for measuring antioxidant capacitywith special emphasis on the dichotomy between competitive and noncompetitivemethods, as well as the dichotomy between kinetic strategies based on oxidationproducts appearance and oxidizable substrate loss.
14
�Laguerre M, Lopez Giraldo LJ, Lecomte J, et al. Chain length affects anti-oxidant properties of chlorogenate esters in emulsion: the cutoff theory behindthe polar paradox. J Agric Food Chem 2009; 57:11335–11342.
This novel work was carried out by means of the CAT method and has reported forthe first time that the relationship between hydrophobicity of phenolic compoundsand their antioxidant capacity (in emulsion) follows a nonlinear trend, which wasconnected to the cut-off effect, well known in biology.
15
�Laguerre M, Lopez Giraldo LJ, Lecomte J, et al. Relationship betweenhydrophobicity and antioxidant ability of ’phenolipids’ in emulsion: a paraboliceffect of the chain length of rosmarinate esters. J Agric Food Chem 2010;58:2869–2876.
By the use of the CAT method, this work confirms with a new homologous series ofamphiphilic phenolics (rosmarinate esters) that the antioxidant capacity increaseswith the increase in the hydrophobicity until a threshold, beyond which any furtherincrement in hydrophobicity leads to a collapse of the antioxidant capacity.
16
�Laguerre M, Lopez Giraldo LJ, Piombo G, et al. Characterization of olive leafphenolics by ESI-MS and evaluation of their antioxidant capacities by the CATassay. J Am Oil Chem Soc 2009; 86:1215–1225.
Example of the use of the CAT method to assess plant extracts (i.e. olive leaves)
17 Chapman RA, Mackay K. The estimation of peroxides in fats and oils by theferric thiocyanate method. J Am Oil Chem Soc 1949; 26:360–363.
18 Shantha NC, Decker EA. Rapid, sensitive, iron-based spectrophotometricmethods for determination of peroxide values of food lipids. J AOAC Int 1994;77:421–424.
Methods for evaluating antioxidants Laguerre et al. 525
19 Mihaljevic B, Katusin-Razem B, Razem D. The reevaluation of the ferricthiocyanate assay for lipid hydroperoxides with special considerations ofthe mechanistic aspects of the response. Free Radic Biol Med 1996; 21:53–63.
20 Jiang ZY, Hunt JV, Wolff SP. Ferrous ion oxidation in the presence of xylenolorange for detection of lipid hydroperoxides in low density lipoproteins. AnalBiochem 1992; 202:384–389.
21 Heath RL, Tappel AL. A new sensitive assay for the measurement of hydro-peroxides. Anal Biochem 1976; 76:184–191.
22
�Bou R, Chen B, Guardiola F, et al. Determination of lipid and proteinhydroperoxides using the fluorescent probe diphenyl-1-pyrenylphosphine.Food Chem 2010 (in press). doi: 10.1016/j.foodchem.2010.05.003
This article described a new method to measure lipid and protein hydroperoxides,which relies on the specific reaction of the phosphine moiety of DPPP with varioushydroperoxides to produce a high-intensity fluorescent DPPP oxide measurable byfluorimetry.
23 Gillam AE, Heilbron IM, Hilditch TP, Morton RA. Spectrographic data ofnatural fats and their fatty acids in relation to vitamin A. Biochem J 1931;25:30–38.
24 Wong SH, Knight JA, Hopfer SM, et al. Lipoperoxides in plasma as measuredby liquid-chromatography separation of malondialdehyde-thiobarbituric acidadduct. Clin Chem 1987; 33:214–220.
25 Tatum VL, Changchit C, Chow CK. Measurement of malondialdehyde byHPLC with fluorescence detection. Lipids 1990; 25:226–229.
26 Dahle LK, Hill EG, Holman RT. The thiobarbituric acid reaction and theautoxidations of polyunsaturated fatty acid methyl esters. Arch BiochemBiophys 1962; 98:253–261.
27 Tirmenstein MA, Pierce CA, Leraas TL, Fariss MW. A fluorescence platereader assay for monitoring the susceptibility of biological samples to lipidperoxidation. Anal Biochem 1998; 265:246–252.
28 Van den Berg JJM, Kuypers FA, Qju JH, et al. The use of cis-parinaric acid todetermine lipid peroxidation in human erythrocyte membranes. Comparison ofnormal and sickle erythrocyte membranes. Biochim Biophys Acta 1988;944:29–39.
29 Simoes APCF, van den Berg JJM, Roelofsen B, Op den Kamp JAF. Lipidperoxidation in Plasmodium falciparum-parasitized human erythrocytes. ArchBiochem Biophys 1992; 298:651–657.
30 De Hingh YCM, Meyer J, Fischer JC, et al. Direct measurement of lipidperoxidation in submitochondrial particles. Biochemistry 1995; 34:12755–12760.
31 Dinis TCP, Almeida LM, Madeira VMC. Lipid peroxidation in sarcoplasmicreticulum membranes: effect on functional and biophysical properties. ArchBiochem Biophys 1993; 301:256–264.
32 Osaka K, Tyurina YY, Dubey RK, et al. Amphotericin B as an intracellularantioxidant: protection against 2,20-azobis(2,4-dimethylvaleronitrile)-inducedperoxidation of membrane phospholipids in rat aortic smooth muscle cells.Biochem Pharmacol 1997; 54:937–945.
33 McGuire SO, James-Kracke MR, Sun GY, Fritsche KL. An esterificationprotocol for cis-parinaric acid-determined lipid peroxidation in immune cells.Lipids 1997; 32:219–226.
34 Steenbergen RGH, Drummen GPC, Op den Kamp JAF, Post JA. The use ofcis-parinaric acid to measure lipid peroxidation in cardiomyocytes duringischemia and reperfusion. Biochim Biophys Acta 1997; 1330:127–137.
35 Ritov VB, Banni S, Yalowich JC, et al. Nonrandom peroxidation of differentclasses of membrane phospholipids in live cells detected by metabolicallyintegrated cis-parinaric acid. Biochim Biophys Acta 1996; 1283:127–140.
36 Zhuang S, Kinsey GR, Yan Y, et al. Extracellular signal-regulated kinaseactivation mediates mitochondrial dysfunction and necrosis induced byhydrogen peroxide in renal proximal tubular cells. J Pharmacol Exp Ther2008; 325:732–740.
37
�Khanim FL, Hayden RE, Birtwistle J, et al. Combined bezafibrateand medroxyprogesterone acetate: potential novel therapy for acutemyeloid leukaemia. PLos One 2009; 4:e8147. doi: 1371/journal.pone.0008147.
This work demonstrates that a combination of bezofibrate and medroxyprogester-one acetate elevated reactive oxygen species (ROS) in acute myeloid leukemiaand delivered the antineoplastic actions of 15d-PGJ2. This finding partly relies onthe use of cPnA to assess lipid peroxidation.
38
�Geetha S, Sai Ram M, Sharma SK, et al. Cytoprotective and antioxidantactivity of seabuckthorn (Hippophae rhamnoides L.) flavones against tert-butylhydroperoxide-induced cytotoxicity in lymphocytes. J Med Food 2009;12:151–158.
Example of the use of cPnA to measure lipid peroxidation in lymphocyte.
39 Laguerre M, Lecomte J, Villeneuve P. Evaluation of the ability of antioxidants tocounteract lipid oxidation: existing methods, new trends and challenges. ProgLipid Res 2007; 46:244–282.
40 Drummen GPC, van Liebergen LCM, op den Kamp JAF, Post JA. C11-BODIPY581/591, an oxidation-sensitive fluorescent lipid peroxidation probe:(micro)spectroscopic characterization and validation of methodology. FreeRadic Biol Med 2002; 33:473–490.
41 Guthrie HD, Welch GR. Use of fluorescence-activated flow cytometry todetermine membrane lipid peroxidation during hypothermic liquid storage andfreeze-thawing of viable boar sperm loaded with 4, 4-difluoro-5-(4-phenyl-1,3-butadienyl)-4-bora-3a, 4a-diaza-s-indaceundecanoic acid. J Anim Sci 2007;85:1402–1411.
42
�Awda BJ, Mackenzie-Bell M, Buhr MM. Reactive oxygen species and boarsperm function. Biol Reprod 2009; 81:553–561.
Example of the use of C11-BODIPY581/591 to measure lipid peroxidation in boarspermatozoa.
43 Ball BA, Vo A. Detection of lipid peroxidation in equine spermatozoa basedupon the lipophilic fluorescent dye C11-BODIPY581/591. J Androl 2002;23:259–269.
44 Aitken RJ, Wingate JK, De Iuliis GN, McLaughlin EA. Analysis of lipidperoxidation in human spermatozoa using BODIPY C11. Mol Hum Reprod2007; 13:203–211.
45 Cosci I, Moretti E, Collodel G. Lipid peroxidation in human spermatozoafrom men with genitourinary infections. Syst Biol Reprod Med 2008; 54:75–83.
46 Drummen GPC, Gadella BM, Post JA, Brouwers JF. Mass spectrometriccharacterization of the oxidation of the fluorescent lipid peroxidation reportermolecule C11-BODIPY581/591. Free Radic Biol Med 2004; 36:1635–1644.
47 Sayes CM, Gobin AM, Ausman KD, et al.Nano-C60 cytotoxicity is due to lipidperoxidation. Biomaterials 2005; 26:7587–7595.
48
��Vernier PT, Levine ZA, Wu YH, et al. Electroporating fields target oxidativelydamaged areas in the cell membrane. PLOS One 2009; 4:e7966;DOI:10.1371/journal.pone.0007966.
This article showed that oxidation of cell membrane enhances the susceptibility ofthe membrane to electropermeabilization, and so, that manipulation of the level ofoxidative stress may lead to efficient electrochemotherapy and electrotransfection-mediated gene therapy. The measurement of oxidative stress at membrane levelwas done using C11-BODIPY581/591.
49 Naguib YMA. A fluorometric method for measurement of peroxyl radicalscavenging activities of lipophilic antioxidants. Anal Biochem 1998; 265:290–298.
50 Drummen GPC, Op den Kamp JAF, Post JA. Validation of the peroxidativeindicators, cis-parinaric acid and parinaroyl-phospholipids, in a model systemand cultured cardiac myocytes. Biochim Biophys Acta 1999; 1436:370–382.
51 Naguib YMA. Antioxidant activities of astaxanthin and related carotenoids.J Agric Food Chem 2000; 48:1150–1154.
52 Makrigiorgos GM, Kassis AI, Mahmood A, et al.Novel fluorescein-based flow-cytometric method for detection of lipid peroxidation. Free Radic Biol Med1997; 22:93–100.
53 Maulik G, Kassis AI, Savvides P, et al. Fluoresceinated phosphoethanolaminefor flow-cytometric measurement of lipid peroxidation. Free Radic Biol Med1998; 26:645–653.
54 Diaz G, Liu S, Isola R, et al. Mitochondrial localization of reactive oxygenspecies by dihydrofluorescein probes. Histochem Cell Biol 2003; 120:319–325.
55 Negre-Salvayre A, Auge N, Duval C, et al. Detection of intracellular reactiveoxygen species in cultured cells using fluorescent probes. Methods Enzymol2002; 352:62–71.
56 Yang J, Liu X, Bhalla K, et al. Prevention of apoptosis by Bcl-2: release ofcytochrome c from mitochondria blocked. Science 1997; 275:1129–1132.
57 Burkitt MJ, Wardman P. Cytochrome c is a potent catalyst of dichlorofluor-escin oxidation: implication for the role of reactive oxygen species in apop-tosis. Biochem Biophys Res Commun 2001; 282:329–333.
58 Hockenbery DM, Oltvai ZN, Yin X-M, et al. Bcl-2 functions in an antioxidantpathway to prevent apoptosis. Cell 1993; 75:241–251.
59 Burton GW, Joyce A, Ingold KV. First proof that vitamin E is a major lipidsoluble, chain-breaking antioxidant in human blood plasma. Lancet 1982;320:327–328.
60 Stocks J, Gutteridge JMC, Sharp RJ, Dormandy TL. The inhibition of lipidautoxidation by human serum and its relationship to serum proteins and alpha-tocopherol. Clin Sci Mol Med 1974; 47:223–233.