Oxidative stress is believed to contribute to the decrease in cellular function that accompanies aging [2] and that is associated with numerous degenerative diseases and even certain types of cancers [3-5]

Cardiolipin (CL) is a phospholipid predominantly found in the mitochondrial inner membrane and associated structurally with individual complexes of the electron transport chain (ETC). Since the ETC is the major mitochondrial reactive oxygen species (ROS) generating site, the proximity to the ETC and bisallylic methylenes of the polyunsaturated fatty acid chains of CL make it a likely target of ROS in the mitochondrial inner membrane. Oxidized cellular CL products, uniquely derived from ROS-induced autoxidation, could serve as biomarkers for the presence of the ROS and help to understand the mechanism of oxidative stress. Since major CL species have four unsaturated acyl chains, while other phospholipids usually have only one on the sn-2 position, characterization of oxidized CL is highly challenging. In the current study we exposed CL, under aerobic conditions, to singlet oxygen (O2), the radical initiator 2,2′-azobis(2methylpropionamidine) dihydrochloride, or room air and the oxidized CL species were characterized by HPLC-MS/MS. Our reversed-phase ion-pair HPLC-MS/MS method can characterize the major and minor oxidized CL species by detecting distinctive fragment ions associated with specific oxidized species. The HPLC-MS/MS results show that monohydroperoxides and bis monohydroperoxides were generated under all three conditions. However, significant amounts of CL dihydroperoxides were produced only by O2-mediated oxidation. These products were barely detectable from radical oxidation either in a liposome bilayer or in thin film. These observations are only possible due to the chromatographic separation of the different oxidized species. 3 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom Introduction The mitochondrial electron transport chain (ETC) is the major site of intracellular reactive oxygen species (ROS) generation (1, 2). The mitochondrially generated ROS are believed to contribute to the decrease in cellular function that accompanies aging (3) and numerous degenerative diseases (4-6). The most abundant ROS generated by mitochondria are superoxide (O2) and hydrogen peroxide (H2O2). Under normal conditions, O2 is disproportionated into O2 and H2O2 by superoxide dismutase and, in turn, H2O2 is disproportionated into H2O and O2 by catalase (7). Under some pathologic conditions, e.g. following ischemic-reperfusion injury, dysfunctional ETC complexes generate elevated levels of superoxide, overwhelming the antioxidant systems (8, 9). Although superoxide and H2O2 are reported to directly cause oxidative damage in biological systems (10, 11), these ROS do not readily react with cardiolipin (CL). The most reactive ROS is the hydroxyl radical, which may be generated by the Fenton reaction, the Haber-Weiss reaction (12) and/or decomposition of peroxynitrite. Recently, evidence has accumulated indicating that singlet oxygen (O2) is generated in vivo and contributes to oxidative stress (13-16). Singlet oxygen is highly reactive and capable of oxidizing many biomolecules (17). Haber-Weiss decomposition of O2 and H2O2 has been reported to generate both hydroxyl radical and O2 (18). Singlet oxygen additionally may be generated by the reaction of H2O2 or lipid hydroperoxides with hypochlorite ion, whose generation by myeloperoxidase has become more fully appreciated (19-21). However it is a great challenge to prove the involvement of any specific ROS in biological systems under oxidative stress. Simply detecting a certain ROS does not necessarily prove its oxidative action, because the ROS detected may have been dispatched by antioxidants 4 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom without causing any damage. Only oxidatively modified products of biomolecules that are unique to certain ROS will provide conclusive evidence of their role in oxidative stress. CL is an unusual phospholipid localized to the mitochondrial inner membrane, where it interacts with proteins of the ETC. CL is required for inner membrane transporters such as the adenine nucleotide translocase (22). Because CL is enriched in polyunsaturated fatty acids, primarily linoleic acid, and is located in close proximity to sites of ROS production in the mitochondrial ETC, it is a primary target for reaction with ROS. Oxidation of CL causes dysfunction of mitochondrial ETC (23) and is proposed to contribute to the release of proapoptotic proteins, including cytochrome c, from the intermembrane space (24, 25). Because of their different chemical reactivities (12), hydroxyl radical and O2 generate different oxidized products in their reactions with proteins (26, 27). In a similar manner, the different ROS could generate uniquely oxidized products of CL which provide important mechanistic information on oxidative stress. However, unlike other phospholipids, the multiple polyunsaturated fatty acids of CL make its oxidized product characterization highly challenging. Previously, we exposed liposomal CL and mitochondria to O2 generated by the photosensitizer, Pc 4, and light, and the oxidized products were analyzed by direct infusion ESIMS/MS (28). This photosensitizer generates a relatively pure source of O2 (29) and CL was suggested as an initial target (30, 31). In the liposome oxidations, we identified two major products with mass increments of +32 and +64 whose MS/MS spectra suggest the existence of at least two isomers for each species. In mitochondria illuminated in the presence of Pc 4, only the +32 species were identified (28). 5 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom In the current study, we exposed CL to O2, the free radical initiator, 2,2′-azobis(2methylpropionamidine) dihydrochloride (AAPH), or room air, and characterized the oxidized CL by reversed-phase ion-pair HPLC-MS/MS. Under the reaction conditions examined, all of these oxidations produced monohydroperoxides and bis monohydroperoxides (CLs containing two monohydroperoxyl chains). Furthermore, only O2 treatment led to formation of significant amounts of dihydroperoxides of CL (CLs containing one dihydroperoxyl chain). The HPLCMS/MS procedure that we developed can separate the three species and partially resolve the isobaric structural isomers in each species, which give rise to different fragmentation patterns detected by MS/MS. Experimental Materials CL and AAPH were purchased from Sigma-Aldrich (St. Louis, MO, USA), dimyristoylphosphatidyl choline (DMPC) from Avanti Polar Lipids (Alabaster, AL, USA), and Whatman TLC plates from Fisher Scientific (Pittsburgh, PA, USA). Pc 4 was a generous gift of Dr. Malcolm E. Kenney (CWRU, Cleveland). Millipore water (18 MΩ) was used throughout. Reversed-phase ion-pair HPLC-MS/MS The reversed-phase ion-pair HPLC-MS/MS system consisted of an HP1100 series quaternary pump with an on-line degasser, autosampler, and column heater (Agilent Technologies, Wilmington, DE). A Symmetry® C18 5μm, 150 x 3.9 mm analytical column (Waters Corporation, Milford MA) was used. Gradient elution used two eluents: eluent A (450 mL acetonitrile, 50 mL water, 2.5 mL triethylamine and 2.5 mL glacial acetic acid) and eluent B (450 mL 2-propanol, 50 mL water, 2.5 mL triethylamine and 2.5 mL glacial acetic acid). The combination of triethylamine and acetic acid in both eluents dynamically forms ion-pairs with 6 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom the negatively charged phosphates in the cardiolipin molecule, resulting in increased chromatographic retention and greatly improved chromatographic resolution. Initially, 50%A 50%B was eluted at a flow rate of 400 μL/min, and this was maintained for 5 min following the injection. Then, a linear gradient to 80% B over 10 min, followed by a gradient to 100% B over 15 min, and finally held at 100% B for 10 min completed the chromatographic run. A 3200 Q TRAP® hybrid triple quadrupole / linear ion trap mass spectrometer, with a Turbo VTM ion source (Applied Biosystems/MDS SCIEX, Concord, Ontario, Canada) was used. The source was operated in the Turbo IonSpray negative ion configuration. The instrument’s linear ion trap mode was employed with an information dependent acquisition method, which included a survey scan in the enhanced MS mode followed by an enhanced product ion scan on the most intense ion in the enhanced MS scan. The enhanced MS scan was performed at a rate of 250 Da/s with a spectral range of 1400-1600 Da, while the enhanced product ion scan was performed at a rate of 1000 Da/s with a spectral range of 100-900 Da. (32) Liposome preparation Vesicles containing DMPC and CL (total 2 mM containing 20% CL) were prepared with a Mini-Extrudor from Avanti Polar Lipids, Inc. (Whatman membrane diameter ≅ 100 nm). Typically, an aliquot of lipid solution in absolute ethanol was evaporated to form a thin film of lipid. PBS (pH = 7.4, 0.1 M NaH2PO4 and K2HPO4, and 0.15 M NaCl) was added to hydrate the film and the lipid mixture was extruded at 45 oC. Incorporation of Pc 4 was achieved by adding a solution of Pc 4 in THF/EtOH (1:1) and incubating the liposome-Pc 4 complex at 45 oC for 30 min with stirring. All procedures were performed while minimizing the exposure of the lipids to air or light. 7 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom Oxidation of CL For O2-mediated oxidation, liposomes containing the photosensitizer, Pc 4, were exposed to 100 mW/cm red light produced by a light-emitting diode array (EFOS, Mississauga, Ontario, Canada; λmax 670–675 nm) at room temperature for 20 min. Radical oxidation of CL was initiated by adding 60 mM AAPH to the liposomes and incubating for 5 min at 37 oC. Air oxidation of CL was performed by exposing a thin film of CL in a test tube to air for 24 h. Lipids were extracted from 0.5 mL of the DMPC+CL liposome solution using 1.5 mL of CHCl3:MeOH (2:1). The extract was dried under a stream of N2 and redissolved in 20 μL of CHCl3. The solution was dispensed on silica gel TLC plates, developed with CHCl3:MeOH:acetic acid:H2O (3: 0.52: 0.36: 0.12) (33) and visualized by I2. The CL spot was scraped into a 0.6-mL microcentrifuge tube and extracted using 100 μL of CHCl3:MeOH (1:1). The conditions for each oxidation were adjusted following preliminary experiments to give similar relative content of oxidized CL species (~30%). Results Characterizing control CL by reversed-phase ion-pair HPLC-MS/MS CL is a phospholipid with a central glycerol connected by phosphodiester linkages at C1 and C3 to two diacylglycerol phosphatidic acid moties. The fragmentation of the singly charged tetralinoleoyl CL negative ion, [M – H] results in fragments observed in the m/z region between 200 and 900 by MS/MS (Figure 1). These peaks and corresponding fragments were reported previously(34, 35). The different relative intensities of the peaks, which are advantageous to our study, are due to the different configurations of the ion traps used (36). The three most intense peaks correspond to free linoleate (m/z 279), monoacylglycerol phosphatidate (m/z 415), and diacylglycerol phosphatidate (m/z 695). Assignments of fragmented oxidized CL products were 8 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom accomplished by examining their mass increments or losses based on these three peaks. Importantly, there are no fragment ions observed from cleavage of the unoxidized linoleic acyl chains from each moiety. O2 -induced CL oxidation analyzed by reversed-phase ion-pair HPLC-MS/MS CL in liposomes was exposed to O2. The chromatogram of CL oxidized by O2 shows unmodified CLs eluting at > 26 min and oxidation products eluting at 22-23, 20-21, and 16-17 min (Figure 2A). Because oxidation decreases the hydrophobicity of the side chain, the CL species suffering the greater oxidation elute earlier. The MS and MS/MS spectra of the analytes eluting around 22-23 min are shown in Figure 2B. These are the least oxidized products. The most abundant ions are singly charged with m/z 1479, 32 Da greater than the [M – H] of tetralinoleoyl CL. To discriminate between hydroperoxides, endoperoxides and dihydroxides modifications, the oxidized CL was treated with a reducing agent (sodium borohydride). This reduction resulted in the elimination of the peak at m/z 1479 with a concomitant increases in the peak at m/z 1463 (-16 from 1479), when analyzed by direct infusion (data not shown). This mass loss is consistent with the reduction of hydroperoxides to hydroxides, which supports the assignment of this CL species to isomers with one hydroperoxyl group. Careful examination of the same chromatographic peak results in the detection of very minor peaks with m/z 1463 in this region attributed to isomeric CLs bearing a single hydroxyl group, showing that hydroxides coelute with hydroperoxides Also at 22-23 min, the peaks in the mass spectrum with m/z 1501 and 1517 are attributed to [M + 2O -2H + Na] and [M + 2O -2H + K], respectively. These precursor ions share the characteristic fragment ions of monohydroperoxides as shown in a typical MS/MS in the inset of Figure 2B. The observed fragment ions at nominal m/z 695 and 727 correspond to the 9 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom unmodified and monohydroperoxyl diacylglycerol phosphatidic acid moieties from the [M + 2O – H]. The m/z 709 ion derives from the dehydration typically observed with lipid hydroperoxides. That this dehydration occurs with the monohydroperoxides and not the underivatized CL and phosphatidic acid supports the conclusion that the loss of water comes from cleavage of the O-O peroxide bond. In the free acyl region (linoleic acid m/z 279), the presence of m/z 293 and barely detectable m/z 311 ions indicate that this dehydration took place to a greater extent during the fragmentation that generates the acyl chain anion. The monoacylglycerol phosphatidic acid fragment ions at m/z 415, 429, and 447 reflect the presence of unmodified and hydroperoxyl fragment ions. The ready loss of water from fragment ions containing hydroperoxides has been previously noted (37, 38). All of the fragment ions are consistent with the assignment of the m/z 1479 precursor as monohydroperoxide isomers of CL. The MS/MS spectrum also shows fragment ions derived from cleavage of hydroperoxylmodified linoleic acyl chains. These acyl chain fragmentations can be detected most readily as neutral losses from the hydroperoxyl-modified diacylglycerol phosphatidic acid fragment. The peaks at m/z 639 (mass loss of 88 Da from 727) and 559 (mass loss of 168 Da from 727) are interpreted as arising from cleavage on the saturated side of the conjugated dienoylhydroperoxide as shown in Figure 3. These mass losses are consistent with the presence of 13and 9-hydroperoxides, respectively, as previously described (39). The MS/MS spectra reveal that the peak at m/z 639 dominates at earlier retention times (Figure 3A) while the peak at m/z 559 is more intense at later times (Figure 3B), indicating that the 13-hydroperoxides, which contain a shorter “alkyl tail” elute earlier than the 9-hydroperoxides. As shown in Figure 2C and D, the major species in the chromatographic peaks at 16-17 and 20-21 min are isobaric species with m/z 1511 interpreted as a [M + 4O –H] ion. Reduction 10 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom of these hydroperoxides with sodium borohydride results in a loss of 32 Da, suggesting that the m/z 1511 ion (Figure 2C and D) corresponds to incorporation of two hydroperoxyl groups in CL (1447). These isobaric species are attributed to CL, in which the hydroperoxyl moieties are on different acyl chains (bis monohydroperoxides) or the hydroperoxyls are on the same linoleoyl chain (dihydroperoxides). The structures of the bis monohydroperoxides and dihydroperoxides were further characterized by MS/MS. Two major isomeric bis monohydroperoxide species can be further differentiated by MS/MS; species with one hydroperoxyl group on each diacylglycerol phosphatidic acid moiety or both hydroperoxyl groups on one diacylglycerol phosphatidic acid moiety. The proposed structures of the fragment ions from these two species observed by MS/MS are shown in Figure 4. The observed characteristic fragment ions for the former are m/z 727 and 709 (Figure 5A), and for the latter m/z 759, 723 and 695 (Figure 5B). However, when the diacylglycerol phosphatidic acid moieties further lose one acyl chain, both isomeric bis monohydroperoxide species will generate the same fragment ions as observed at m/z 447, 429, 415, 311, 293, and 279. It was found that the intensities of ions at m/z 727 and 709 are higher than those with m/z 695 and 759 at the earlier retention time (Figure 5), suggesting CL species with hydroperoxyl groups on each diacylglycerol phosphatidic acid moiety have shorter retention times than the species with both hydroperoxyl groups on one diacylglycerol phosphatidic acid moiety. The observation of a peak with m/z 359 (mass loss of 88 from 447) suggests the existence of the species with a hydroperoxyl group on the 13 position. Close examination of the MS spectra of the eluting chromatographic peaks revealed that both m/z 1511 peaks in Figure 2 C and D coeluted with barely detectable m/z 1495 peaks, whose MS/MS spectrum suggests modification of the parent CL by one hydroxyl and one hydroperoxyl 11 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom group. A CL species with m/z 1477 found in Figure 2D, predicted to be derived from hydroperoxyl CL(18:2)3(18:3)1, also eluted in the region of the chromatogram containing these dihydroperoxides, indicating that the additional unsaturation had a similar effect on retention time as the addition of the second hydroperoxyl group. The key feature of the MS/MS spectrum of the chromatographic peak at 20-21 min in Figure 2D, with the precursor ion of m/z 1511, is the lack of any characteristic fragment ions derived from monohydroperoxyl acyl chains, namely m/z 727, 709, 447, 429, 311, or 293. The m/z 723 ion (inset) resulted from loss of two water molecules from dihydroperoxyl diacylglycerol phosphatidic acid, and fragment ions at m/z 588, 599, 613, and 629 derived from cleavage of a dihydroperoxyl linoleic acyl chain, strongly support the assigned dihydroperoxide structure for the modified CLs eluting as the major species at this time (Figure 2D). Although the peaks at m/z 599 and 613 may be generated from fragmentation of 10,12-dihydroperoxides and the peak at m/z 588 from 9,12-dihydroperoxides (Figure 6), these assignments, without precedent MS/MS data, remain tentative until confirmed by synthesis of authentic material or other characterizations. We speculate that the presence of the easily fragmented acyl chain containing two hydroperoxyl groups may be responsible for the low intensity for peaks of the corresponding diacylglycerol phosphatidic acid, monoacylglycerol phosphatidic acid and free linoleate. Free radical-initiated oxidation of CL Free radical-initiated oxidation of CL gives +32 and +64 as major oxidized products observed by MS analysis. Aerobic radical initiated oxidation generated significant amounts of monohydroperoxides and bis monohydroperoxides but no observable dihydroperoxides as shown in the HPLC-MS total ion chromatogram of Figure 7A. 12 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom The MS spectrum of the peak at 22-23 min showed two major species with m/z 1479 and 1463 (Figure 7B), suggesting the presence of significant amounts of hydroperoxides as well as hydroxides. The formation of hydroxides was found to occur during the preparation of vesicles, and the relative intensity of the peak decreased as the peaks of hydroperoxides increased by the radical-induced oxidation. Addition of a chelating agent, diethylene triamine pentaacetic acid, did not reduce the intensity of the peak at m/z 1463 or affect oxidized products of CL (data not shown). The MS/MS spectrum of the same chromatographic peak shows the characteristic fragment ions from monohydroperoxides also found in O2-generated monohydroperoxides. The ions derived from the cleavage of the linoleic acyl chain, (ions at m/z 640, 359, and 559) support the assertion that the major species are 13 and 9-hydroperoxides. The MS spectrum of the chromatographic peak at 16-17 min also contains hydroxyl species, although bis monohydroperoxides still constitute the most prominent ions (Figure 7C). The peak with m/z 1479 suggests that bis monohydroxides coeluted at this retention time. MS/MS spectra of the same chromatographic peak contains all of the characteristic fragment ions of bis monohydroperoxides, ions with m/z 728, 710, 447, 429, and 293, and bis monohydroxides, observable ions with m/z 712 and 431. The positions of the hydroperoxide modifications are suggested to be at C13 and C9 by the peaks with m/z 640, 359, and 559. The peaks at m/z 728 and 760 suggest that free radical oxidation also can generate both species with both hydroperoxyl groups on one glycerol moiety and one hydroperoxyl group on each glycerol moiety as shown in Figure 4. There is a very small chromatographic peak at 20 min with a m/z 1477, predicted to be hydroperoxyl CL(18:2)3(18:3)1. Fragment ions observed in the MS/MS spectrum of this peak are consistent with this oxidized CL species as noted earlier for Figure 2D. The accumulated MS 13 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom spectrum of this region of the chromatogram also revealed a barely detectable peak at m/z 1511, whose molecular weight corresponds to dihydroperoxides. With extended reaction time (20 min), the intensity of the peak at m/z 1511 increased with concomitant increases in the intensities of the other oxidized species of CL. However the intensity of the peak at m/z 1511 is still negligible and the signal-to-noise ratio of the peak is less than 3. CL oxidation by room air Exposing a dried film of CL to air for 24 h also produced a similar amount of oxidized species through autoxidation. The major products observed by HPLC-MS/MS were monohydroperoxide and bis monohydroperoxide species, without any significant amount of hydroxide species (Figure 8). Similar MS/MS spectra of both chromatographic peaks at 18-19 and 24-25 min suggest that air oxidation generates the same monohydroperoxides and dihydroperoxides products as the other two ROS, with no significant dihydroperoxides. Discussion Reversed-phase ion-pair HPLC-MS/MS analysis of CL The chromatograms of oxidized CL clearly showed that only O2 generated significant amounts of all three major species of oxidized products, while radical reaction generated only monohydroperoxides and bis monohydroperoxides (Scheme 1). The chromatographic separation of the three species of oxidized products was necessary to make this determination, and the inclusion of a chromatographic component in our methodology is fundamental to our approach. The general observation has been made that analysis by mass spectrometry alone can yield incorrect results, due to the presence of unknown products generating unanticipated fragment ions resulting in false positive results (40). In our specific case, while the isobaric isomers of oxidized CL are indistinguishable by mass, these same compounds can be chromatographically 14 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom resolved and structurally characterized as we have demonstrated in Figures 2 and 7. Although the observed corresponding characteristic fragment ions and consistent chromatographic retention times of each species strongly support the structures as proposed, further characterizations of physically separated individual oxidized products and analysis of synthesized authentic standards will be necessary to differentiate the detailed structures and quantify the relative yields of the many species suggested by the chromatographic results. Responsible ROS; radical vs. O2 Superoxide and H2O2 are the primary ROS generated by the mitochondrial ETC. Although certain oxidative damage caused by superoxide and H2O2 has been reported, (10, 11) these ROS do not readily react with biomolecules, especially CL. Rather, hydroxyl radical, derived from superoxide and H2O2 by a Fenton-type or Haber-Weiss reaction is considered to be the main ROS responsible for most cellular oxidative damage (12). The hydroxyl radical is considered the most reactive ROS found in biological systems. Nonetheless, there has been increasing evidence suggesting a role for O2 in various forms of oxidative stress, e.g., ischemiareperfusion (13, 41, 42), aging associated mitochondrial DNA lesions (43), and UV-A mediated skin damage (15, 43). In spite of the fact that several mechanisms have been proposed for generation of O2 in biological systems and the reactivity of O2 towards biomolecules has been demonstrated by in vitro studies, there is still a lack of direct evidence for involvement of O2 in any of the forms of oxidative stress. In biological systems, simply detecting certain ROS may not be sufficient to prove its role in oxidative stress, because the ROS detected may be dispatched by antioxidants or converted into more reactive ROS (or reactive nitrogen species) depending on the microenvironment around the ROS generated. The amount of ROS does not necessarily correlate 15 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom with the degree of oxidative damage (44). Therefore, oxidized products of biomolecules uniquely derived from certain ROS may provide conclusive evidence to identify the responsible ROS. Dihydroperoxides, generated in this unambiguous model system using O2, may be the chemotype of O2. The presence of dihydroperoxides is convincingly demonstrated from these data only under O2-mediated oxidation but not under radical oxidation. Since the extent of oxidized CL found both in vivo and in vitro experiments is moderate (45-48), our approach, where about 30% of CL was oxidized, is sufficient to identify these products. However, we can not rule out the possibility that radical-mediated oxidation could generate significant amounts of dihydroperoxides. The conditions used for radical oxidation, e.g., concentration of AAPH, reaction time, or temperature, may not be optimal for dihydroperoxides to accumulate, or the steady state favors only low concentrations of dihydroperoxides in the presence of a continuous radical flux. Additional experimental examination of the generation and/or decomposition of individual dihydroperoxide species under various conditions will be required to resolve these questions. These investigations also may lead to the detection of specific dihydroperoxide isomers which will serve as unequivocal biomarkers for O2. An additional intriguing result of these studies is the absence of any chain cleaved CL oxidation products. In vivo aldehydes, e.g. 4-hydroxynonenal, and other thiobarbituric acid reactive substances derived from linoleic acid oxidation have been used as monitors of oxidative stress. These products are readily generated from linoleic acid in the presence of a one electron reductant, routinely reduced metal ions like Fe(II) (49, 50). The results of our studies suggest that production of aldehyde byproducts requires, in addition to oxygen radicals and/or singlet oxygen, a source of electrons to reduce the initial hydroperoxides. Reaction mechanism for dihydroperoxides 16 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom The result that O2 generates significant amounts of dihydroperoxides, whereas free radical oxidation does not, may be attributable to different reaction mechanisms of these two ROS. One chemical rationale for this differential reactivity comes from considering the structure of the monohydroperoxides. The initial step of oxidation by free radicals with a linoleic acyl chain is abstraction of hydrogen from the bis allylic carbon. The resulting dienoyl radical reacts more readily at the 9 or 13 position, resulting in 9or 13monohydroperoxyls, which subsequently abstract a H-atom from a donor. The stability of the conjugated dienehydroperoxide will hinder the further hydrogen abstraction from this acyl group (51, 52). Rather free radicals will abstract a hydrogen from a more reactive bisallylic methylene of another acyl chain. This phenomenon will be more significant in biological systems where the amount of free radical is limited. This contrasts with the behavior of singlet oxygen-mediated oxidation. Because singlet oxygen reacts readily with conjugated dienes, the rate constant for reaction with 2,4-hexadiene is faster than that for reaction with methyl linoleate (53, 54). These differences in chemical selectivity would favor formation of dihydroperoxides with singlet oxygen. A second chemical selectivity difference is in the observed product distribution when singlet oxygen reacts with methyl linoleate in solution, where 10and 12-hydroperoxy linoleic methyl esters, in addition to the 9and 13-hydroperoxy isomers, are generated (39, 55). These authors suggested the potential of 10and 12-hydroperoxy linoleate as biomarkers for O2 (55-57). These isomers may be intermediates for the formation of dihydroperoxides from O2-mediated oxidation of CL. Interestingly, characteristic fragment ions corresponding to 10or 12monohydroperoxides were not detected by MS/MS, suggesting that the second peroxidation occurred faster than the first peroxidation on the acyl chain. Alternatively, the dihydroperoxides 17 by gest, on O cber 0, 2017 w w w .j.org D ow nladed fom may be generated by different mechanisms, such as incorporation of two oxygen molecules at the same time or involving rearrangement of 9or 13-hydroperoxides to 10or 12hydroperoxides. In any case, the fact that the oxidized products of the linoleic acid side chains of CL, present in a liposome bilayer, are different from the oxidation products detected from methyl linoleate oxidation in solution suggests that the intramolecular interaction between the linoleic acyl chains may be an important contributor to oxidation mechanisms in the bilayer. It is still possible that 10and 12hydroperoxides may have lower ionization efficiencies or higher resistances to acyl chain cleavage. In conclusion, we demonstrate by reverse-phase ion-pair HPLC-MS/MS that O2 preferentially generates significant amounts of dihydroperoxides. Detection of CL dihydroperoxides species in biological systems may be the chemotype of O2. Acknowledgement We thank Prof. Nancy Oleinick for sharing her equipment and technique to generate Pc 4mediated O2. This work was supported by NIH/NIA grant (P01 AG015885). 18bygest,onOcber0,2017www.j.orgDownladedfom References1. Storz, P. 2006. Reactive oxygen species-mediated mitochondria-to-nucleus signaling: a keyto aging and radical-caused diseases. Sci STKE 2006: re3.2. Hoffmann, S., D. Spitkovsky, J. P. Radicella, B. Epe, and R. J. Wiesner. 2004. Reactiveoxygen species derived from the mitochondrial respiratory chain are not responsible for thebasal levels of oxidative base modifications observed in nuclear DNA of mammalian cells.Free Radic Biol Med 36: 765-773.3. Finkel, T., and N. J. Holbrook. 2000. Oxidants, oxidative stress and the biology of ageing.Nature 408: 239-247.4. Smith, M. A., C. A. Rottkamp, A. Nunomura, A. K. Raina, and G. Perry. 2000. Oxidativestress in Alzheimer's disease. Biochim Biophys Acta 1502: 139-144.5. Wallace, D. C. 2001. A mitochondrial paradigm for degenerative diseases and ageing.Novartis Found Symp 235: 247-263; discussion 263-246.6. Toyokuni, S., K. Okamoto, J. Yodoi, and H. Hiai. 1995. Persistent oxidative stress in cancer.FEBS Lett 358: 1-3.7. Kowaltowski, A. J., N. C. de Souza-Pinto, R. F. Castilho, and A. E. Vercesi. 2009.Mitochondria and reactive oxygen species. Free Radic Biol Med 47: 333-343. 8. Zimmerman, M. C., and I. H. Zucker. 2009. Mitochondrial dysfunction and mitochondrialproduced reactive oxygen species: new targets for neurogenic hypertension? Hypertension53: 112-114.9. Marin-Garcia, J., Y. Pi, and M. J. Goldenthal. 2006. Mitochondrial-nuclear cross-talk in the aging and failing heart. Cardiovasc Drugs Ther 20: 477-491. 19bygest,onOcber0,2017www.j.orgDownladedfom 10. Fridovich, I. 1986. Biological effects of the superoxide radical. Arch Biochem Biophys 247:1-11.11. Ramasarma, T. 1982. Generation of H2O2 in biomembranes. Biochim Biophys Acta 694: 69-93.12. Girotti, A. W. 1998. Lipid hydroperoxide generation, turnover, and effector action inbiological systems. J Lipid Res 39: 1529-1542.13. Toufektsian, M. C., F. R. Boucher, S. Tanguy, S. Morel, and J. G. de Leiris. 2001. Cardiactoxicity of singlet oxygen: implication in reperfusion injury. Antioxid Redox Signal 3: 63-69.14. Lee, J. W., H. Miyawaki, E. V. Bobst, J. D. Hester, M. Ashraf, and A. M. Bobst. 1999.Improved functional recovery of ischemic rat hearts due to singlet oxygen scavengershistidine and carnosine. J Mol Cell Cardiol 31: 113-121.15. Grether-Beck, S., S. Olaizola-Horn, H. Schmitt, M. Grewe, A. Jahnke, J. P. Johnson, K.Briviba, H. Sies, and J. Krutmann. 1996. Activation of transcription factor AP-2 mediatesUVA radiationand singlet oxygen-induced expression of the human intercellular adhesionmolecule 1 gene. Proc Natl Acad Sci U S A 93: 14586-14591.16. Prado, F. M., M. C. Oliveira, S. Miyamoto, G. R. Martinez, M. H. Medeiros, G. E. Ronsein, and P. Di Mascio. 2009. Thymine hydroperoxide as a potential source of singlet molecularoxygen in DNA. Free Radic Biol Med 47: 401-409.17. Davies, M. J. 2003. Singlet oxygen-mediated damage to proteins and its consequences. Biochem Biophys Res Commun 305: 761-770. 18. Khan, A. U., and M. Kasha. 1994. Singlet molecular oxygen in the Haber-Weiss reaction.Proc Natl Acad Sci U S A 91: 12365-12367. 20bygest,onOcber0,2017www.j.orgDownladedfom 19. Nicholls, S. J., and S. L. Hazen. 2009. Myeloperoxidase, modified lipoproteins, andatherogenesis. J Lipid Res 50 Suppl: S346-351.20. Pitt, A. R., and C. M. Spickett. 2008. Mass spectrometric analysis of HOCland free-radical-induced damage to lipids and proteins. Biochem Soc Trans 36: 1077-1082.21. Nicholls, S. J., L. Zheng, and S. L. Hazen. 2005. Formation of dysfunctional high-densitylipoprotein by myeloperoxidase. Trends Cardiovasc Med 15: 212-219.22. Hoffmann, B., A. Stockl, M. Schlame, K. Beyer, and M. Klingenberg. 1994. Thereconstituted ADP/ATP carrier activity has an absolute requirement for cardiolipin as shownin cysteine mutants. J Biol Chem 269: 1940-1944.23. Petrosillo, G., G. Casanova, M. Matera, F. M. Ruggiero, and G. Paradies. 2006. Interactionof peroxidized cardiolipin with rat-heart mitochondrial membranes: induction ofpermeability transition and cytochrome c release. FEBS Lett 580: 6311-6316.24. Ott, M., J. D. Robertson, V. Gogvadze, B. Zhivotovsky, and S. Orrenius. 2002. Cytochromec release from mitochondria proceeds by a two-step process. Proc Natl Acad Sci U S A 99:1259-1263.25. Gonzalvez, F., J. J. Bessoule, F. Rocchiccioli, S. Manon, and P. X. Petit. 2005. Role ofcardiolipin on tBid and tBid/Bax synergistic effects on yeast mitochondria. Cell Death