Next Article in Journal
Regulation of Cellular Ribonucleoprotein Granules: From Assembly to Degradation via Post-translational Modification
Next Article in Special Issue
Effects of Air Pollution on Cellular Senescence and Skin Aging
Previous Article in Journal
Salmonella Promotes Its Own Survival in B Cells by Inhibiting Autophagy
Previous Article in Special Issue
Age-Related Lysosomal Dysfunctions
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Cells
Volume 11
Issue 13
10.3390/cells11132059
cells-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Article

Dual Oxidase, a Hydrogen-Peroxide-Producing Enzyme, Regulates Neuronal Oxidative Damage and Animal Lifespan in Drosophila melanogaster

by
Minwoo Baek
,
Wijeong Jang
and
Changsoo Kim
*
School of Biological Sciences and Technology, Chonnam National University, Gwangju 61186, Korea
*
Author to whom correspondence should be addressed.
Cells 2022, 11(13), 2059; https://doi.org/10.3390/cells11132059
Submission received: 28 May 2022 / Revised: 23 June 2022 / Accepted: 27 June 2022 / Published: 29 June 2022
(This article belongs to the Special Issue Controversies and Recent Advances in Senescence and Aging)
Browse Figures
Versions Notes

Abstract

:
Reducing the oxidative stress in neurons extends lifespan in Drosophila melanogaster, highlighting the crucial role of neuronal oxidative damage in lifespan determination. However, the source of the reactive oxygen species (ROS) that provoke oxidative stress in neurons is not clearly defined. Here, we identify dual oxidase (duox), a calcium-activated ROS-producing enzyme, as a lifespan determinant. Due to the lethality of duox homozygous mutants, we employed a duox heterozygote that exhibited normal appearance and movement. We found that duox heterozygous male flies, which were isogenized with control flies, demonstrated extended lifespan. Neuronal knockdown experiments further suggested that duox is crucial to oxidative stress in neurons. Our findings suggest duox to be a source of neuronal oxidative stress associated with animal lifespan.

1. Introduction

Hydrogen peroxide (H2O2) is a reactive oxygen species (ROS) that functions in signaling pathways by specifically oxidizing redox-sensitive proteins in diverse biological processes [1,2,3,4]. However, the upregulated or dysregulated production of H2O2 in combination with diminished anti-ROS activity confers oxidative stress that abrogates redox-dependent signaling or nonspecifically and irreversibly damages macromolecules, in turn accelerating the aging process and decreasing lifespan [5,6,7,8,9]. Neurons are particularly susceptible to oxidative stress, and the elevation of the antioxidant power in neurons has been shown to extend lifespan [10,11,12,13,14]. Various anti-ROS enzymes and anti-ROS transcriptional networks are well known, yet the source of ROS production that provokes oxidative stress in neurons is not yet completely understood.
ROS production is inducible by members of the NADPH oxidase (NOX) family; such induced production is distinct from the steady-state ROS production that occurs through oxidative respiration in mitochondria [15]. Dual oxidase (Duox) is a member of the Nox family, with an EF-hand motif that is activated by intracellular calcium to produce H2O2 [1,16,17]. It is widely expressed in the nervous system in rats, zebrafish, and Drosophila [18,19,20,21]. Inflammation, wounds, and various signals that increase intracellular calcium ion concentration all activate duox [22,23,24,25] and, in particular, UV irradiation, ROS, and p38 MAPK signaling increase its expression [18,26,27,28,29,30]. Duox is known to mediate pain hypersensitivity due to UV-induced damage [31] and, in the CNS, axon regeneration after wounds [32,33]. However, the full role of duox in the nervous system still remains largely unknown. In Drosophila, there is only a single duox gene, in contrast to the two genes present in mammals [21]. Here, we show that through its generation of H2O2, duox contributes to oxidative stress in neurons and is a determinant of Drosophila melanogaster lifespan.

2. Materials and Methods

2.1. Fly Strains and Maintenance

Tub-Gal4, elav-Gal4, Mef-Gal4, UAS-duoxRNAi (#38907 and #32903), and duoxKG07745 were purchased from the Bloomington Drosophila Stock Center. UAS-duoxRNAi (#38907 and #32903) and duoxKG07745 were outcrossed with w1118 for ten generations to eliminate background effects. Flies were raised on standard cornmeal fly food at 25 °C and 50% humidity in a 12-hour light/dark-cycle incubator.

2.2. Lifespan and Oxidative Stress Assays

For lifespan assays, 20 flies per vial were transferred to fresh food vials every two days. Dead flies were counted every day. For survival under oxidative stress, 5-day-old flies were starved for 6 h at 25 °C in vials containing water-soaked tissues and then transferred to vials containing either normal food with 5 mM methyl viologen hydrate (paraquat) or 5% sucrose-agar medium with 5% hydrogen peroxide [34]. Dead flies were counted every 12 h.

2.3. Locomotive Activity

Negative geotactic movement assays were performed as described previously [35]. Briefly, a vial (9.5 cm × 2 cm) containing 10 flies was tapped to send the flies to the bottom. Flies that crossed the 8-centimeter line from the bottom within 10 s were scored. In total, 100 male flies were assessed in 10 vials (10 flies per vial).

2.4. RT-PCR and Real-Time PCR

Total RNA was extracted from 20 flies using Trizol reagent (Invitrogen, Grand Island, NY, USA) and cDNA was obtained by reverse transcription (TOPscript RT Mix; Enzynomics, Seoul, Korea). Real-time PCR was conducted using SYBR green PCR Master Mix on the ABI PRISM 7500 system (Applied Biosystem, Foster City, CA, USA). The primer pairs used were as follows. Duox: CAGACCGAGAAACAGCGCTAC, AAACAGCCGGCTGAGCCTGCG; rp49: CACCAGGAACTTCTTGAATCCGG, AGATCGTGAAGAAGCGCACC; catalase: CGGCTTCCAATCAGTTGAT, GATGTGAACTTCCTGGATGAG; dSOD1:CAAGGGCACGGTTTTCTTC, TCCGGACCGCACTTCAATC; dSOD2: AATTTCGCAAACTGCAAGC, ACCACCAAGCTGATTCAGC.

2.5. Determination of Total ROS Levels

Total ROS was measured as previously described [36]. Briefly, 10 flies or the heads of 50 flies were homogenized in 200 μL of 50 mM Tris-HCl, pH 7.4, on ice. Extracts were centrifuged at 13,200 rpm for 10 min at 4 °C. Homogenates were incubated with H2DCFDA (Life Technologies, Carlsbad, CA, USA) at 5 μM in a 200-microliter reaction volume at 37 °C for 15 min in darkness, carried out on 96-well plates. Florescence intensity was monitored on a Gemini XPS fluorescence microplate reader (Molecular Devices, Sunnyvale, CA, USA) set for 488 nm excitation and 520 nm emission. Florescence intensity was normalized by protein amount measured by Bradford method [37]. All experiments were carried out with three biological replicates.

2.6. Determination of H2O2 Levels

H2O2 was measured as previously described [36]. Briefly, 10 flies were homogenized in phosphate saline buffer (50 mM, pH 7.4) containing aminotriazol (2 mg/mL) and incubated at 4 °C for 15 min. The extracts were centrifuged at 13,200 rpm for 10 min at 4 °C to obtain supernatants. H2O2 levels were measured using a hydrogen peroxide assay kit (Cayman Chemical, Ann Arbor, MI, USA) on a microplate reader (VersaMax; Molecular Devices) set to 590 nm. H2O2 levels were normalized according to protein amount measured by Bradford method [37]. All experiments were carried out with three biological replicates.

2.7. Determination of Protein Oxidation

Carbonyl groups in proteins were detected using an oxyblot protein oxidation detection kit (Milipore, Billerica, MA, USA) according to the manufacturer’s instructions. Briefly, proteins were extracted from 10 flies or ~50 fly heads using RIPA buffer, reacted with 2,4-dinitophenylhydrazine (5 mM) at 25 °C for 100 min, and then subjected to SDS/PAGE and Western blotting using an antibody to the dinitrophenyl moiety. The blots were developed with ECL (Amersham, Buckinghamshire, UK) and the images were captured with a Vilber Lourmat Fusion FX (Vilber Lourmat, Eberhardzell, Baden-Württemberg, Germany). Band intensities were determined with the Fusion program (Vilber Lourmat). Finally, blots were stripped with a stripping buffer (Thermo Fisher scientific, Waltham, MA, USA), and then by a separate Western blot carried out using β-actin antibody (Santa Cruz, Dallas, TX, USA), which was used as loading control. All experiments were carried out with three biological replicates.

2.8. Determination of DNA Oxidation

The level of 8-hydroxydeomyguanosine (8-OHdG) was measured using the OxiSelectTM Oxidative DNA Damage ELISA kit (Cell Biolabs, San Diego, CA, USA). Briefly, genomic DNA from 10 flies or ~50 fly heads was extracted using PureLinkTM genomic DNA kits (Invitrogen, Carlsbad, CA, USA), treated at 95 °C for 5 min, and digested with nuclease P1 (20 mM sodium acetate, pH 5.2) and alkaline phosphatase (100 mM Tris, pH 7.5). Samples were centrifuged for 5 min at 6000× g and the supernatants were used for ELISA assays following the manufacturer’s instructions. The amount of 8-OHdG in each sample was calculated based on an 8-OHdG standard curve.

2.9. TUNEL Labeling

Adult fly brains were dissected in M3 medium (Merck, Boston, MA, USA), fixed in 4% paraformaldehyde in phosphate buffered saline (PBS, 50 mM, pH 7.4) for 20 min at room temperature, washed with PBS, and permeabilized by 2 min incubation in PBS containing Triton X-100 (0.1%) on ice. After washing with PBS three times, the samples were first incubated in Na citrate (0.1 M, pH 6.0) for 10 min at 65 °C, followed by incubation in Tris-HCl buffer (0.1 M, pH 7.5) containing 3% BSA and 20% bovine serum albumin for 30 min. After washing three times with PBS, the samples were incubated in TUNEL assay solution (In Situ Cell Death Detection Kit; Roche, Basel, Switzerland) for 1 h at 37 °C, in accordance with the manufacturer’s recommendations. After washing three times with PBS, the samples were mounted in mounting solution (Prolong Gold Antifade reagent; Life Technologies) and examined by confocal microscopy (Leica TCS SP5; Leica Microsystems, Morrisville, NC, USA).

2.10. Statistical Analysis

The statistical significance of differences in standard error of the mean (SEM) values was obtained using Student’s t-test (two-tailed), analysis of variance (ANOVA) with post hoc analysis (Dunnett’s tests, two-tailed). Kaplan-Meier survival curves were used for lifespan and survival analysis with log-rank tests. Prism software (GraphPad version 6.0, San Diego, CA, USA) was used to calculate p-values. Results were considered statistically significant at levels * p < 0.05, ** p < 0.01, *** p < 0.001, and **** p < 0.0001.

3. Results

To find genes involved in lifespan extension, we carried out a small-scale screening of mutants with extended lifespan, which identified duox heterozygous (duoxKG07745/+) male flies of interest. In the transgenic allele, the P-element KG07745 was inserted into the second intron of the duox locus, which reduced the duox transcripts to ~half the level in control flies (Figure 1A–C). As the insertion was downstream of the initiation codon, the Duox protein structure was disrupted, suggesting that the duoxKG07745 allele was probably null or severely hypomorphic with regards to protein function The. DuoxKG07745 homozygotes were lethal, while the duoxKG07745 heterozygotes were normal in both appearance and movement (Figure S1).
Initial screening involved a small number (n = 40) of unisogenized duox heterozygous males. To ensure rigor, we isogenized the duox heterozygous flies with the control flies (w1118) ten times to reduce genetic background differences, and increased the population to 400 flies, with 20 flies per vial given fresh food every two days. We focused on the duox heterozygous male flies due to the small effect of the allele on the lifespans of the heterozygous female flies (Figure S2A). The control male flies (w1118) lived for a median of 70 days; meanwhile, the isogenized duox heterozygous males had an extended median lifespan of 81 days, which was an increase of 15% (Figure 1D, Table S1). Next, we employed the bipartite Gal4/UAS expression system to knock down the duox function across the whole body, including in both muscle and neurons. Rigorously, we isogenized the UAS-duoxRNAi (#38907, 32903) flies with w1118 flies ten times to reduce the genetic background differences between the Gal4 > UAS-duoxRNAi flies and the control Gal4 > w1118 flies. Driving the whole-body duoxRNAi (#38907 and #32903) expression with the whole-body Gal4 (tub-Gal4) was lethal. A second experiment using muscle-only Gal4 (mef-Gal4) did not demonstrate pronounced lifespan extension in the males or females (Figure S2C,D). However, driving the duox RNAi with the pan-neuronal Gal4 (elav-Gal4) extended the male lifespan by 10% and 20%, respectively, for the duoxRNAi #38907 and #32903 relative to the elav-Gal4/+ control (Figure 1E, Table S1); the lifespan extension in the females was not pronounced (Figure S2B).
As Duox is a ROS-producing enzyme, the duox heterozygotes (duox+/−) would be expected to produce less ROS than the control flies (duox+/+). The global ROS was measured using the non-fluorescent compound 2′,7′-dichlorodihydrofluorescein diacetate (DCFH-DA), which reacted with the ROS to produce fluorescent dichlorofluorescein (DCF). The ROS-dependent DCF fluorescence intensity was normalized to the protein concentration in each extract. The whole-fly extracts from the duox heterozygotes produced less ROS than those from the controls (Figure 2A). The head extracts from the flies with the neuronal knockdown of the duox also exhibited less ROS than the controls (Figure 2B). Similarly, the assays of the H2O2 production revealed that the duox heterozygote whole-fly extracts produced less H2O2 than those from the controls (Figure 2C). The same was true of the head extracts from the flies with the neuronal knockdown of the duox (Figure 2D). ROS mediates the oxidation of amino acid residues in proteins and of the bases in DNA [38,39,40], and this oxidation was decreased in the whole-body extracts of the duox heterozygous male flies (Figure 3A,C). Similarly, the neuronal knockdown of the duox via RNAi resulted in reduced protein and DNA oxidation in the head extracts (Figure 3B,D).
Given that the duox heterozygous males experienced less oxidative damage, next, we examined whether these males exhibited increased survival when provided with ROS-producing food. When given food-containing paraquat, an agent that produces cellular ROS, the duoxKG07745 heterozygous males exhibited increased survival; they also showed increased survival on H2O2-containing food (Figure 4A,B). Oxidative stress is relevant to apoptotic cell death and neurodegeneration, suggesting that apoptotic cells might be reduced by duox reduction. Indeed, the apoptotic cells in the brain were reduced by the duox heterozygosity and by its neuronal knockdown (Figure S3). The observed ROS decrease could have been due to increased levels of anti-ROS enzymes. However, the levels of the anti-ROS enzyme catalase, dSOD1, and dSOD2 were constant with age regardless of the duox status (Figure S4), suggesting that the lower ROS level in the duox heterozygous flies was not due to anti-ROS enzymes, but to duox heterozygosity.

4. Discussion

Neurons are vulnerable to oxidative stress, which is related to neuronal aging, neuropathies, and lifespan. Considerable attention has been paid to antioxidant defense systems, but the ROS sources that oxidize macromolecules in neurons are not yet well defined. Here, we identify Duox, a calcium-activated NADPH oxidase, as a determinant of neuronal oxidative stress and lifespan. We found that neuronal oxidative damage was reduced and lifespan was extended by the neuronal knockdown of duox in Drosophila melanogaster. Our findings suggest that duox is a source of ROS production in neurons, which affects lifespan.
It is intriguing that oxidative stress, particularly stress in neurons, should impact lifespan. It was previously shown that lifespan can be extended by enhancing anti-oxidative power in neurons, specifically through the neuronal overexpression of Peroxiredoxin 4 (prx4), an anti-ROS protein, and of glutamate-cysteine ligase, an enzyme that catalyzes the biosynthesis of the reducing agent, glutathione [13,41]. Similarly, the neuronal knockdown of Kelch-like ECH-associated protein 1 (keap1) increases longevity [8,12]; this gene encodes an inhibitor of the cap ’n’ collar (CncC) transcription factor, the Drosophila homolog of the mammalian nuclear factor E2-related factor 2 (NRF2), which provides a major anti-ROS cellular system by directly inducing expression of anti-ROS genes. Thus, our findings are in line with previous reports that reducing oxidative stress in neurons is beneficial to lifespan.
We further observed that lifespan extension is pronounced in duox heterozygous males but less so in heterozygous females, and a similar trend was seen with the neuronal knockdown of the duox. Such sexual dimorphism in longevity has previously been observed in other contexts. For example, increased reducing power in neurons via the increased activation of CncC due to keap1 mutation results in extended lifespan for males, but not females [42]. A recent report similarly found that oltipraz, an NRF2-activating drug, extends lifespan more in males than in females [43]. It appears that sexual dimorphism exists in regard to neuronal oxidative-stress-dependent lifespan.
It is worth mentioning the duox-dependent lifespan extension in C. elegans. In this model nematode, lifespan is expectably shortened upon the substantive increase of duox activity [44]. However, and much more unexpectedly, a modest increase in duox results in extended lifespan [44,45]. Why is a low-level increase in duox activity beneficial to lifespan? The underlying mechanism involves the activation of the expression of SKN-1, the C. elegans homolog of NRF2 [44]. NRF2 is a transcription factor that responds to ROS and is known to extend lifespan [9,45,46,47]. Therefore, extension of lifespan with a low-level increase in duox is achieved by strengthening anti-ROS power via NRF2 activation. Thus, our findings concerning Drosophila duox in combination with other reports regarding C. elegans duox support the notion that oxidative stress regulates lifespan.
Oxidative stress can occur due to an imbalance between ROS production and the cellular antioxidant defense network. In Drosophila, NRF2-dependent anti-ROS power declines with age, suggesting that oxidative stress is more likely to occur in older animals [8,43,48,49]. Duox activity and expression are increased in gut and embryo epithelial cells undergoing apoptotic cell death, in mammalian neurons through the stabilization of duox transcripts by ROS, and in gut epithelial cells by PLCβ-calcium and p38 MAPK signaling [18,24,27,29,30]. In addition, duox is elevated in aged brains and in Drosophila models of Alzheimer’s disease [50]. Thus, chronic inflammation, protein-aggregate-induced cell death, and various signals involving PLCβ-calcium or p38 MAK could aberrantly activate duox activity and expression in neurons, which could confer oxidative stress and lifespan determination. It would be informative to examine whether neuronal duox knockdown reduces neuronal inflammation, a hallmark of which is the activation of microglial cells or astrocytes. However, the pursuit of this idea is hindered by the lack of antibodies or markers for activated microglial and astrocytic cells, which is a limitation of these studies.

Supplementary Materials

The following supporting information can be downloaded at: https://www.mdpi.com/article/10.3390/cells11132059/s1, Figure S1. Negative geotactic movement. Wild-type (duox+/+) and duox heterozygous (duox+/−) male flies were used for negative geotactic movement. n = 100 (10 flies/vial, total 10 vials for each point). duox+/+ denotes w1118 flies. duox+/− denotes duox kG07745/+ flies, which were isogenized with control (w1118) flies. Figure S2. Lifespan of female (A–C) and male flies (D). (A) Wild-type and duox heterozygous flies. n = 400, female flies. duox+/+ denotes w1118 flies. duox+/− denotes duox kG07745/+ flies, which were isogenized with control (w1118) flies. (B,C) Lifespan of elav-Gal4>UAS-duoxRNAi (elav/#38907, 32903) and mef-Gal4> UAS-duoxRNAi (mef/#38907, 32903). n = 200, female flies. (D) Lifespan of mef-Gal4> UAS-duoxRNAi (mef/#38907, 32903). n = 200, male flies. UAS-duoxRNAi (#38907, 32903) flies were isogenized with control w1118 flies ten times to reduce genetic background differences. Figure S3. Decrease of TUNEL-positive cells in the brain with duox heterozygosity and neuronal duox reduction. (A,B) Confocal images of whole-mount staining of Drosophila (40-day-old) brains with the DNA dye DAPI (blue) and TUNEL (red). (C,D) Quantification of TUNEL-positive cells in panels A & B. Error bars represent SEM of three replicates. Student’s t-test, *** p < 0.001. duox+/+ and duox+/− denote w1118 and duox+/kG07745, respectively. elav/#38907, 32903 denotes elav-Gal4/ UAS-duoxRNAi #38907, elav-Gal4/+; UAS-duoxRNAi #32903/+; Figure S4. Anti-ROS enzyme levels are not affected by duox heterozygosity. Agarose gel images of RT-PCR products of anti-ROS genes obtained from male flies. Similar results were obtained among the three replicates. dSOD denotes Drosophila superoxide dismutase. rp49 was used as a loading control. +/+ and +/− denote w1118 and duox+/kG07745, respectively. Table S1. Quantification of Lifespan.

Author Contributions

Conceptualization, M.B. and C.K. Experiments, M.B. and W.J. Writing, M.B. and C.K. All authors have read and agreed to the published version of the manuscript.

Funding

This work was supported by grants from the National Research Foundation of Korea (NRF-2021R1A2C1010334 to CK, NRF-2020R1I1A1A01074292 to WJ).

Acknowledgments

We thank the Bloomington Drosophila Stock Center and Vienna Drosophila RNAi Center for flies.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Bedard, K.; Krause, K.H. The NOX Family of ROS-Generating NADPH Oxidases: Physiology and Pathophysiology. Physiol. Rev. 2007, 87, 245–313. [Google Scholar] [CrossRef] [PubMed]
  2. Zhang, J.; Wang, X.; Vikash, V.; Ye, Q.; Wu, D.; Liu, Y.; Dong, W. ROS and ROS-mediated cellular signaling. Oxid. Med. Cell. Longev. 2016, 2016, 4350965. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  3. Sies, H. Hydrogen peroxide as a central redox signaling molecule in physiological oxidative stress: Oxidative eustress. Redox Biol. 2017, 11, 613–619. [Google Scholar] [CrossRef]
  4. Holmström, K.M.; Finkel, T. Cellular mechanisms and physiological consequences of redox-dependent signalling. Nat. Rev. Mol. Cell Biol. 2014, 15, 411–421. [Google Scholar] [CrossRef] [PubMed]
  5. Van der Vliet, A.; Janssen-Heininger, Y.M. Hydrogen peroxide as a damage signal in tissue injury and inflammation: Murderer, mediator, or messenger? J. Cell. Biochem. 2014, 115, 427–435. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  6. Colavitti, R.; Finkel, T. Reactive Oxygen Species as Mediators of Cellular Senescence. IUBMB Life 2005, 57, 277–281. [Google Scholar] [CrossRef]
  7. Sohal, R.S.; Orr, W.C. The redox stress hypothesis of aging. Free Radic. Biol. Med. 2012, 52, 539–555. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  8. Rahman, M.M.; Sykiotis, G.P.; Nishimura, M.; Bodmer, R.; Bohmann, D. Declining signal dependence ofNrf2-MafS-regulated gene expression correlates with aging phenotypes. Aging Cell 2013, 12, 554–562. [Google Scholar] [CrossRef] [Green Version]
  9. Kubben, N.; Zhang, W.; Wang, L.; Voss, T.C.; Yang, J.; Qu, J.; Liu, G.-H.; Misteli, T. Repression of the Antioxidant NRF2 Pathway in Premature Aging. Cell 2016, 165, 1361–1374. [Google Scholar] [CrossRef] [Green Version]
  10. Rego, A.C.; Oliveira, C.R. Mitochondrial dysfunction and reactive oxygen species in excitotoxicity and apoptosis: Implications for the pathogenesis of neurodegenerative diseases. Neurochem. Res. 2003, 28, 1563–1574. [Google Scholar] [CrossRef] [Green Version]
  11. Liu, Z.; Zhou, T.; Ziegler, A.C.; Dimitrion, P.; Zuo, L. Oxidative Stress in Neurodegenerative Diseases: From Molecular Mechanisms to Clinical Applications. Oxid. Med. Cell. Longev. 2017, 2017, 2525967. [Google Scholar] [CrossRef]
  12. Spiers, J.G.; Breda, C.; Robinson, S.; Giorgini, F.; Steinert, J.R. Drosophila Nrf2/Keap1 Mediated Redox Signaling Supports Synaptic Function and Longevity and Impacts on Circadian Activity. Front. Mol. Neurosci. 2019, 12, 86. [Google Scholar] [CrossRef] [PubMed]
  13. Orr, W.C.; Radyuk, S.; Prabhudesai, L.; Toroser, D.; Benes, J.J.; Luchak, J.M.; Mockett, R.J.; Rebrin, I.; Hubbard, J.G.; Sohal, R.S. Overexpression of Glutamate-Cysteine Ligase Extends Life Span in Drosophila melanogaster. J. Biol. Chem. 2005, 280, 37331–37338. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  14. Wang, M.C.; Bohmann, D.; Jasper, H. JNK Signaling Confers Tolerance to Oxidative Stress and Extends Lifespan in Drosophila. Dev. Cell 2003, 5, 811–816. [Google Scholar] [CrossRef] [Green Version]
  15. Buvelot, H.; Jaquet, V.; Krause, K.H. Mammalian NADPH Oxidases. Methods Mol. Biol. 2019, 1982, 17–36. [Google Scholar] [CrossRef]
  16. De Deken, X.; Corvilain, B.; Dumont, J.E.; Miot, F. Roles of DUOX-Mediated Hydrogen Peroxide in Metabolism, Host Defense, and Signaling. Antioxid. Redox Signal. 2014, 20, 2776–2793. [Google Scholar] [CrossRef]
  17. Geiszt, M.; Witta, J.; Baffi, J.; Lekstrom, K.; Leto, T.L. Dual oxidases represent novel hydrogen peroxide sources supporting mucosal surface host defense. FASEB J. 2003, 17, 1–14. [Google Scholar] [CrossRef]
  18. Damiano, S.; Fusco, R.; Morano, A.; De Mizio, M.; Paternò, R.; De Rosa, A.; Spinelli, R.; Amente, S.; Frunzio, R.; Mondola, P.; et al. Reactive Oxygen Species Regulate the Levels of Dual Oxidase (Duox1-2) in Human Neuroblastoma Cells. PLoS ONE 2012, 7, e34405. [Google Scholar] [CrossRef]
  19. Weaver, C.J.; Leung, Y.F.; Suter, D.M. Expression dynamics of NADPH oxidases during early zebrafish development. J. Comp. Neurol. 2015, 524, 2130–2141. [Google Scholar] [CrossRef]
  20. Conner, G.E. Regulation of dual oxidase hydrogen peroxide synthesis results in an epithelial respiratory burst. Redox Biol. 2021, 41, 101931. [Google Scholar] [CrossRef]
  21. Kim, S.H.; Lee, W.J. Role of DUOX in gut inflammation: Lessons from Drosophila model of gut-microbiota interactions. Front. Cell. Infect. Microbiol. 2014, 3, 116. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  22. Razzell, W.; Evans, I.R.; Martin, P.; Wood, W. Calcium Flashes Orchestrate the Wound Inflammatory Response through DUOX Activation and Hydrogen Peroxide Release. Curr. Biol. 2013, 23, 424–429. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  23. Sirokmány, G.; Pató, A.; Zana, M.; Donkó, Á.; Bíró, A.; Nagy, P.; Geiszt, M. Epidermal growth factor-induced hydrogen peroxide production is mediated by dual oxidase 1. Free Radic. Biol. Med. 2016, 97, 204–211. [Google Scholar] [CrossRef] [Green Version]
  24. Ha, E.M.; Lee, K.A.; Park, S.H.; Kim, S.H.; Nam, H.J.; Lee, H.Y.; Kang, D.; Lee, W.J. Regulation of DUOX by the Galphaq-phospholipase Cbeta-Ca2+ pathway in Drosophila gut immunity. Dev. Cell. 2009, 16, 386–397. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  25. Juarez, M.T.; Patterson, R.A.; Sandoval-Guillen, E.; McGinnis, W. Duox, Flotillin-2, and Src42A Are Required to Activate or Delimit the Spread of the Transcriptional Response to Epidermal Wounds in Drosophila. PLoS Genet. 2011, 7, e1002424. [Google Scholar] [CrossRef] [Green Version]
  26. Xiao, X.; Huang, M.; Fan, C.; Zuo, F. DUOX2 participates in skin aging induced by UVB in HSF2 cells by activating NF-kappaB signaling. Exp. Ther. Med. 2021, 21, 157. [Google Scholar] [CrossRef]
  27. Ha, E.M.; Lee, K.A.; Seo, Y.Y.; Kim, S.H.; Lim, J.H.; Oh, B.H.; Kim, J.; Lee, W.J. Coordination of multiple dual oxidase-regulatory pathways in responses to commensal and infectious mi-crobes in drosophila gut. Nat. Immunol. 2009, 10, 949–957. [Google Scholar] [CrossRef]
  28. Kizhedathu, A.; Chhajed, P.; Yeramala, L.; Sain Basu, D.; Mukherjee, T.; Vinothkumar, K.R.; Guha, A. Duox-generated reactive oxygen species activate ATR/Chk1 to induce G2 arrest in Drosophila tra-cheoblasts. eLife 2021, 10, e68636. [Google Scholar] [CrossRef]
  29. Fogarty, C.E.; Diwanji, N.; Lindblad, J.L.; Tare, M.; Amcheslavsky, A.; Makhijani, K.; Brückner, K.; Fan, Y.; Bergmann, A. Extracellular Reactive Oxygen Species Drive Apoptosis-Induced Proliferation via Drosophila Macro-phages. Curr. Biol. 2016, 26, 575–584. [Google Scholar] [CrossRef] [Green Version]
  30. Amcheslavsky, A.; Lindblad, J.L.; Bergmann, A. Transiently “Undead” Enterocytes Mediate Homeostatic Tissue Turnover in the Adult Drosophila Midgut. Cell Rep. 2020, 33, 108408. [Google Scholar] [CrossRef]
  31. Jang, W.; Baek, M.; Han, Y.S.; Kim, C. Duox mediates ultraviolet injury-induced nociceptive sensitization in Drosophila larvae. Mol. Brain 2018, 11, 16. [Google Scholar] [CrossRef] [Green Version]
  32. Rieger, S.; Sagasti, A. Hydrogen Peroxide Promotes Injury-Induced Peripheral Sensory Axon Regeneration in the Zebrafish Skin. PLoS Biol. 2011, 9, e1000621. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  33. Yang, L.Q.; Chen, M.; Ren, D.L.; Hu, B. Dual Oxidase Mutant Retards Mauthner-Cell Axon Regeneration at an Early Stage via Modulating Mito-chondrial Dynamics in Zebrafish. Neurosci. Bull. 2020, 36, 1500–1512. [Google Scholar] [CrossRef] [PubMed]
  34. Slack, C.; Werz, C.; Wieser, D.; Alic, N.; Foley, A.; Stocker, H.; Withers, D.J.; Thornton, J.M.; Hafen, E.; Partridge, L. Regulation of Lifespan, Metabolism, and Stress Responses by the Drosophila SH2B Protein, Lnk. PLoS Genet. 2010, 6, e1000881. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  35. Ali, Y.O.; Escala, W.; Ruan, K.; Zhai, R.G. Assaying Locomotor, Learning, and Memory Deficits in Drosophila Models of Neurodegeneration. J. Vis. Exp. 2011, 49, e2504. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  36. Casani, S.; Gómez-Pastor, R.; Matallana, E.; Paricio, N. Antioxidant compound supplementation prevents oxidative damage in a Drosophila model of Parkinson’s disease. Free Radic. Biol. Med. 2013, 61, 151–160. [Google Scholar] [CrossRef]
  37. Bradford, M.M. A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein-dye binding. Anal. Biochem. 1976, 72, 248–254. [Google Scholar] [CrossRef]
  38. Korolainen, M.A.; Nyman, T.; Nyyssonen, P.; Hartikainen, E.S.; Pirttila, T. Multiplexed Proteomic Analysis of Oxidation and Concentrations of Cerebrospinal Fluid Proteins in Alzheimer Disease. Clin. Chem. 2007, 53, 657–665. [Google Scholar] [CrossRef] [Green Version]
  39. Smith, M.A.; Sayre, L.M.; Anderson, V.E.; Harris, P.L.; Beal, M.F.; Kowall, N.; Perry, G. Cytochemical Demonstration of Oxidative Damage in Alzheimer Disease by Immunochemical Enhancement of the Carbonyl Reaction with 2,4-Dinitrophenylhydrazine. J. Histochem. Cytochem. 1998, 46, 731–735. [Google Scholar] [CrossRef] [Green Version]
  40. Furukawa, A.; Hiraku, Y.; Oikawa, S.; Luxford, C.; Davies, M.J.; Kawanishi, S. Guanine-specific DNA damage induced by gamma-irradiated histone. Biochem. J. 2005, 388 Pt 3, 813–818. [Google Scholar] [CrossRef] [Green Version]
  41. Klichko, V.I.; Orr, W.C.; Radyuk, S.N. The role of peroxiredoxin 4 in inflammatory response and aging. Biochim. Biophys. Acta (BBA)-Mol. Basis Dis. 2015, 1862, 265–273. [Google Scholar] [CrossRef] [PubMed]
  42. Sykiotis, G.P.; Bohmann, D. Keap1/Nrf2 signaling regulates oxidative stress tolerance and lifespan in Drosophila. Dev. Cell 2008, 14, 76–85. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  43. Cheng, Y.; Pitoniak, A.; Wang, J.; Bohmann, D. Preserving transcriptional stress responses as an antiaging strategy. Aging Cell 2021, 20, e13297. [Google Scholar] [CrossRef] [PubMed]
  44. Sasakura, H.; Moribe, H.; Nakano, M.; Ikemoto, K.; Takeuchi, K.; Mori, I. Lifespan extension by peroxidase/dual oxidase-mediated ROS signaling through pyrroloquinoline quinone in C. elegans. J. Cell Sci. 2017, 130, 2631–2643. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  45. Ewald, C.Y.; Hourihan, J.M.; Bland, M.S.; Obieglo, C.; Katic, I.; Mazzeo, L.E.M.; Alcedo, J.; Blackwell, T.K.; Hynes, N.E. NADPH oxidase-mediated redox signaling promotes oxidative stress resistance and longevity through memo-1 in C. elegans. eLife 2017, 6, e19493. [Google Scholar] [CrossRef] [PubMed]
  46. Blackwell, T.K.; Steinbaugh, M.J.; Hourihan, J.M.; Ewald, C.Y.; Isik, M. SKN-1/Nrf, stress responses, and aging in Caenorhabditis elegans. Free Radic. Biol. Med. 2015, 88, 290–301. [Google Scholar] [CrossRef] [Green Version]
  47. Castillo-Quan, J.I.; Li, L.; Kinghorn, K.J.; Ivanov, D.K.; Tain, L.S.; Slack, C.; Kerr, F.; Nespital, T.; Thornton, J.; Hardy, J.; et al. Lithium Promotes Longevity through GSK3/NRF2-Dependent Hormesis. Cell. Rep. 2016, 15, 638–650. [Google Scholar] [CrossRef] [Green Version]
  48. Przybysz, A.J.; Choe, K.P.; Roberts, L.J.; Strange, K. Increased age reduces DAF-16 and SKN-1 signaling and the hormetic response of Caenorhabditis elegans to the xenobiotic juglone. Mech. Ageing Dev. 2009, 130, 357–369. [Google Scholar] [CrossRef] [Green Version]
  49. Ungvari, Z.; Bailey-Downs, L.; Gautam, T.; Sosnowska, D.; Wang, M.; Monticone, R.E.; Telljohann, R.; Pinto, J.T.; de Cabo, R.; Sonntag, W.E.; et al. Age-associated vascular oxidative stress, Nrf2 dysfunction, and NF-κB activation in the nonhuman primate Macaca mulatta. J. Gerontol. A Biol. Sci. Med. Sci. 2011, 66, 866–875. [Google Scholar] [CrossRef]
  50. Barati, A.; Masoudi, R.; Yousefi, R.; Monsefi, M.; Mirshafiey, A. Tau and amyloid beta differentially affect the innate immune genes expression in Drosophila models of Alzheimer’s disease and β-D Mannuronic acid (M2000) modulates the dysregulation. Gene 2021, 808, 145972. [Google Scholar] [CrossRef]
Cells 11 02059 g001 550
Figure 1. Extension of male lifespan with duox heterozygosity and neuronal duox knockdown. (A) Diagram showing the location of the P-element (KG07745), which is inserted in the second intron of duox. Empty and filled squares denote noncoding and coding regions of exons, respectively. Arrows denote primers used for RT-PCR. (B) Agarose-gel image of RT-PCR products following amplification of the duox gene from control (w1118, denoted duox+/+) and heterozygous (duox KG07745/+, denoted duox+/−) flies. rp49 was used as a loading control. Three independent experiments carried out with similar results. (C) qRT-PCR of duox gene, with rp-49 used as a control. Relative expression denotes duox transcript level. Averages and standard errors were derived from three independent experiments. Student’s t-test, *** p < 0.001. (D) Lifespan of wild-type and duox heterozygous male flies. Twenty flies/vial, total twenty vials. Log-rank test, **** p< 0.0001. duox+/+ denotes w1118 flies. duox+/− denotes duox+/kG07745 flies, which were isogenized ten times with control flies (w1118). (E) Lifespans of elav-Gal4 > UAS-duoxRNAi flies. elav/#38907 and elav/#32903 denote elav-Gal4 > UAS-duoxRNAi #38907, elav-Gal4/+; UAS-duoxRNAi #32903/+. Twenty flies/vial, total ten vials, male flies. Log-rank test, **** p < 0.0001. UAS-duoxRNAi (#38907, 32903) flies were isogenized with control w1118 flies ten times to reduce genetic background differences.
Figure 1. Extension of male lifespan with duox heterozygosity and neuronal duox knockdown. (A) Diagram showing the location of the P-element (KG07745), which is inserted in the second intron of duox. Empty and filled squares denote noncoding and coding regions of exons, respectively. Arrows denote primers used for RT-PCR. (B) Agarose-gel image of RT-PCR products following amplification of the duox gene from control (w1118, denoted duox+/+) and heterozygous (duox KG07745/+, denoted duox+/−) flies. rp49 was used as a loading control. Three independent experiments carried out with similar results. (C) qRT-PCR of duox gene, with rp-49 used as a control. Relative expression denotes duox transcript level. Averages and standard errors were derived from three independent experiments. Student’s t-test, *** p < 0.001. (D) Lifespan of wild-type and duox heterozygous male flies. Twenty flies/vial, total twenty vials. Log-rank test, **** p< 0.0001. duox+/+ denotes w1118 flies. duox+/− denotes duox+/kG07745 flies, which were isogenized ten times with control flies (w1118). (E) Lifespans of elav-Gal4 > UAS-duoxRNAi flies. elav/#38907 and elav/#32903 denote elav-Gal4 > UAS-duoxRNAi #38907, elav-Gal4/+; UAS-duoxRNAi #32903/+. Twenty flies/vial, total ten vials, male flies. Log-rank test, **** p < 0.0001. UAS-duoxRNAi (#38907, 32903) flies were isogenized with control w1118 flies ten times to reduce genetic background differences.
Cells 11 02059 g001
Cells 11 02059 g002 550
Figure 2. Decrease in global ROS and H2O2 levels with duox heterozygosity and neuronal duox knockdown. Global ROS (A,B) and H2O2 (C,D) levels normalized to protein concentration were derived for whole-fly extracts (A,C) and head extracts (B,D). Values for duox+/+ (A,C) and elav/+ (B,D) were set to 100%. Error bars represent SEM of three replicates using 5-day-old male flies. Student’s t-test, * p < 0.05, ** p < 0.01, *** p < 0.001. duox+/+ and duox+/− denote w1118 and duox+/kG07745. elav/#38907, 32903 denotes elav-Gal4/UAS-duoxRNAi #38907, elav-Gal4/+; UAS-duoxRNAi #32903/+.
Figure 2. Decrease in global ROS and H2O2 levels with duox heterozygosity and neuronal duox knockdown. Global ROS (A,B) and H2O2 (C,D) levels normalized to protein concentration were derived for whole-fly extracts (A,C) and head extracts (B,D). Values for duox+/+ (A,C) and elav/+ (B,D) were set to 100%. Error bars represent SEM of three replicates using 5-day-old male flies. Student’s t-test, * p < 0.05, ** p < 0.01, *** p < 0.001. duox+/+ and duox+/− denote w1118 and duox+/kG07745. elav/#38907, 32903 denotes elav-Gal4/UAS-duoxRNAi #38907, elav-Gal4/+; UAS-duoxRNAi #32903/+.
Cells 11 02059 g002
Cells 11 02059 g003 550
Figure 3. Decrease in oxidative damage with duox heterozygosity and neuronal duox knockdown. Relative protein and DNA oxidation levels in whole-fly extracts (A,C) and in head extracts (B,D). Data were set to duox+/+ (A,C) and elav/+ (B,D) at 100%. Error bars represent SEM of three replicates using 60-day-old (A) and 45-day-old male flies (B–D). Three replicates. Error bars represent SEM. Student’s t-test, * p < 0.05, ** p < 0.01, and *** p < 0.001. duox+/+ and duox+/− denote w1118 and duox+/kG07745, respectively. elav/#38907, 32903 denotes elav-Gal4/ UAS-duoxRNAi #38907, elav-Gal4/+; UAS-duoxRNAi #32903/+.
Figure 3. Decrease in oxidative damage with duox heterozygosity and neuronal duox knockdown. Relative protein and DNA oxidation levels in whole-fly extracts (A,C) and in head extracts (B,D). Data were set to duox+/+ (A,C) and elav/+ (B,D) at 100%. Error bars represent SEM of three replicates using 60-day-old (A) and 45-day-old male flies (B–D). Three replicates. Error bars represent SEM. Student’s t-test, * p < 0.05, ** p < 0.01, and *** p < 0.001. duox+/+ and duox+/− denote w1118 and duox+/kG07745, respectively. elav/#38907, 32903 denotes elav-Gal4/ UAS-duoxRNAi #38907, elav-Gal4/+; UAS-duoxRNAi #32903/+.
Cells 11 02059 g003
Cells 11 02059 g004 550
Figure 4. ROS resistance associated with duox heterozygosity. Survival of 5-day-old male flies on food containing 10 mM paraquat (A) and 10% hydrogen peroxide (H2O2) (B). n = 200 (20 flies/vial, total 10 vials). Log-rank test, **** p < 0.0001. duox+/+ denotes w1118 flies. duox+/− denotes duox+/kG07745 flies, which were isogenized ten times with control flies (w1118).
Figure 4. ROS resistance associated with duox heterozygosity. Survival of 5-day-old male flies on food containing 10 mM paraquat (A) and 10% hydrogen peroxide (H2O2) (B). n = 200 (20 flies/vial, total 10 vials). Log-rank test, **** p < 0.0001. duox+/+ denotes w1118 flies. duox+/− denotes duox+/kG07745 flies, which were isogenized ten times with control flies (w1118).
Cells 11 02059 g004
Publisher’s Note: MDPI stays neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Share and Cite

MDPI and ACS Style

Baek, M.; Jang, W.; Kim, C. Dual Oxidase, a Hydrogen-Peroxide-Producing Enzyme, Regulates Neuronal Oxidative Damage and Animal Lifespan in Drosophila melanogaster. Cells 2022, 11, 2059. https://doi.org/10.3390/cells11132059

AMA Style

Baek M, Jang W, Kim C. Dual Oxidase, a Hydrogen-Peroxide-Producing Enzyme, Regulates Neuronal Oxidative Damage and Animal Lifespan in Drosophila melanogaster. Cells. 2022; 11(13):2059. https://doi.org/10.3390/cells11132059

Chicago/Turabian Style

Baek, Minwoo, Wijeong Jang, and Changsoo Kim. 2022. "Dual Oxidase, a Hydrogen-Peroxide-Producing Enzyme, Regulates Neuronal Oxidative Damage and Animal Lifespan in Drosophila melanogaster" Cells 11, no. 13: 2059. https://doi.org/10.3390/cells11132059

APA Style

Baek, M., Jang, W., & Kim, C. (2022). Dual Oxidase, a Hydrogen-Peroxide-Producing Enzyme, Regulates Neuronal Oxidative Damage and Animal Lifespan in Drosophila melanogaster. Cells, 11(13), 2059. https://doi.org/10.3390/cells11132059

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop