47 research outputs found

    Biochemical comparison of venoms from young Colombian Crotalus durissus cumanensis and their parents

    Full text link
    Crotalus durissus cumanensis, a rattlesnake endemic to Colombia and Venezuela, is considered one of the most lethal snake species in Latin America. The aim of the present study was to compare the protein content and biological activity of the venom obtained from eight specimens of C. durissus cumanensis, namely two adults from different localities of Colombia and six offspring born in captivity. Protein profiles of crude venoms were analyzed by SDS-PAGE and RP-HPLC, and biological activities were evaluated for lethality, edema, defibrination, hemolytic and coagulant activities to assess individual venoms of adults and a pool of young snake venoms. Transient edema appeared rapidly after venom inoculation, whereas hemorrhagic effect was not observed. Differences in protein profiles, lethality, hemolytic, coagulant and defibrinating activities between both adult snake venoms were observed; those from the mother snake exhibited higher activities. Venoms from young snakes were similar to the one obtained from the mother, but the coagulant effect was stronger in offspring venoms. Notably, biological effects of the father snake venom were not comparable to those previously described for C. durissus cumanensis from Venezuela and C. durissus terrificus from Brazil, confirming the high variability of the venom from Crotalus species

    Expression of two barley proteinase inhibitors in tomato promotes endogenous defensive response and enhances resistance to Tuta absoluta

    Get PDF
    [EN] Background: For as long as 350 million years, plants and insects have coexisted and developed a set of relationships which affect both organisms at different levels. Plants have evolved various morphological and biochemical adaptations to cope with herbivores attacks. However, Tuta absoluta (Meyrick) (Lepidoptera: Gelechiidae) has become the major pest threatening tomato crops worldwide and without the appropriated management it can cause production losses between 80 to 100%. Results: The aim of this study was to investigate the in vivo effect of a serine proteinase inhibitor (BTI-CMe) and a cysteine proteinase inhibitor (Hv-CPI2) from barley on this insect and to examine the effect their expression has on tomato defensive response. We found that larvae fed on the double transgenic plants showed a notable reduction in weight. Moreover, only 56% of the larvae reached the adult stage. The emerged adults showed wings deformities and reduced fertility. We also investigated the effect of proteinase inhibitors ingestion on the insect digestive enzymes. Our results showed a decrease in larval trypsin activity. Transgenes expression had no harmful effect on Nesidiocoris tenuis (Reuter) (Heteroptera: Miridae), a predator of Tuta absoluta, despite transgenic tomato plants attracted the mirid. We also found that barley cystatin expression promoted plant defense by inducing the expression of the tomato endogenous wound inducible Proteinase inhibitor 2 (Pin2) gene, increasing the production of glandular trichomes and altering the emission of volatile organic compounds. Conclusion: Our results demonstrate the usefulness of the co-expression of different proteinase inhibitors for the enhancement of plant resistance to Tuta absoluta.This work was partly supported by grants BIO2013-40747-R and AGL2014-55616-C3 from the Spanish Ministry of Economy and Competitiveness (MINECO)Hamza, R.; Pérez-Hedo, M.; Urbaneja, A.; Rambla Nebot, JL.; Granell Richart, A.; Gaddour, K.; Beltran Porter, JP.... (2018). Expression of two barley proteinase inhibitors in tomato promotes endogenous defensive response and enhances resistance to Tuta absoluta. BMC Plant Biology. 18. https://doi.org/10.1186/s12870-018-1240-6S18Oerke EC. Crop losses to pests. J Agric Sci. 2005;144(01):31.Jouanin L, Bonadé-Bottino M, Girard C, Morrot G, Giband M. Transgenic plants for insect resistance. Plant Sci. 1998;131(1):1–11.Markwick NP, Docherty LC, Phung MM, Lester MT, Murray C, Yao JL, Mitra DS, Cohen D, Beuning LL, Kutty-Amma S, et al. Transgenic tobacco and apple plants expressing biotin-binding proteins are resistant to two cosmopolitan insect pests, potato tuber moth and lightbrown apple moth, respectively. Transgenic Res. 2003;12(6):671–81.Koiwa H, Bressan RA, Hasegawa PM. Regulation of protease inhibitors and plant defense. Trends Plant Sci. 1997;2(10):379–84.Ryan CA. Protease inhibitors in plants: genes for improving defenses against insects and pathogens. Annu Rev Phytopathol. 1990;28(1):425–49.Abdeen A, Virgos A, Olivella E, Villanueva J, Aviles X, Gabarra R, Prat S. Multiple insect resistance in transgenic tomato plants over-expressing two families of plant proteinase inhibitors. Plant Mol Biol. 2005;57(2):189–202.Quilis J, López-García B, Meynard D, Guiderdoni E, San Segundo B. Inducible expression of a fusion gene encoding two proteinase inhibitors leads to insect and pathogen resistance in transgenic rice. Plant Biotechnol J. 2014;12(3):367–77.Smigocki AC, Ivic-Haymes S, Li H, Savic J. Pest protection conferred by a Beta vulgaris serine proteinase inhibitor gene. PLoS One. 2013;8(2):e57303.Mazumdar-Leighton S, Broadway RM. Transcriptional induction of diverse midgut trypsins in larval Agrotis ipsilon and Helicoverpa zea feeding on the soybean trypsin inhibitor. Insect Biochem Mol Biol. 2001;31(6–7):645–57.Oppert B, Morgan TD, Hartzer K, Kramer KJ. Compensatory proteolytic responses to dietary proteinase inhibitors in the red flour beetle, Tribolium castaneum (Coleoptera: Tenebrionidae). Comparative Biochemistry and Physiology Part C: Toxicology & Pharmacology. 2005;140(1):53–8.Broadway RM. Dietary regulation of serine proteinases that are resistant to serine proteinase inhibitors. J Insect Physiol. 1997;43(9):855–74.Zhu-Salzman K, Koiwa H, Salzman R, Shade R, Ahn JE. Cowpea bruchid Callosobruchus maculatus uses a three-component strategy to overcome a plant defensive cysteine protease inhibitor. Insect Mol Biol. 2003;12(2):135–45.Oppert B, Morgan TD, Hartzer K, Lenarcic B, Galesa K, Brzin J, Turk V, Yoza K, Ohtsubo K, Kramer KJ. Effects of proteinase inhibitors on digestive proteinases and growth of the red flour beetle, Tribolium castaneum (Herbst) (Coleoptera: Tenebrionidae). Comparative biochemistry and physiology Toxicology & pharmacology : CBP. 2003;134(4):481–90.Duan X, Li X, Xue Q, Abo-El-Saad M, Xu D, Wu R. Transgenic rice plants harboring an introduced potato proteinase inhibitor II gene are insect resistant. Nat Biotechnol. 1996;14(4):494–8.Pompermayer P, Lopes AR, Terra WR, Parra JRP, Falco MC, Silva-Filho MC. Effects of soybean proteinase inhibitor on development, survival and reproductive potential of the sugarcane borer, Diatraea saccharalis. Entomologia Experimentalis et Applicata. 2001;99(1):79–85.Alfonso-Rubí J, Ortego F, Castañera P, Carbonero P, Díaz I. Transgenic expression of trypsin inhibitor CMe from barley in indica and japonica rice, confers resistance to the rice weevil Sitophilus oryzae. Transgenic Res. 2003;12(1):23–31.Altpeter F, Diaz I, Mc Auslane H, Gaddour K, Carbonero P, Vasil IK. Increased insect resistance in transgenic wheat stably expressing trypsin inhibitor CMe. Mol Breed. 1999;5(1):53–63.Martinez M, Cambra I, Carrillo L, Diaz-Mendoza M, Diaz I. Characterization of the entire cystatin gene family in barley and their target cathepsin L-like cysteine-proteases, partners in the hordein mobilization during seed germination. Plant Physiol. 2009;151(3):1531–45.FAOSTAT: Food and Organization of the United Nations, statistics division. 2017.Mueller LA, Lankhorst RK, Tanksley SD, Giovannoni JJ, White R, Vrebalov J, Fei Z, van Eck J, Buels R, Mills AA, et al. A snapshot of the emerging tomato genome sequence. The Plant Genome. 2009;2(1):78–92.Ellul P, Garcia-Sogo B, Pineda B, Rios G, Roig L, Moreno V. The ploidy level of transgenic plants in agrobacterium-mediated transformation of tomato cotyledons (Lycopersicon esculentum L. mill.) is genotype and procedure dependent. Theor Appl Genet. 2003;106(2):231–8.Pino LE, Lombardi-Crestana S, Azevedo MS, Scotton DC, Borgo L, Quecini V, Figueira A, Peres LE. The Rg1 allele as a valuable tool for genetic transformation of the tomato'Micro-Tom'model system. Plant Methods. 2010;6(1):23.Sharma MK, Solanke AU, Jani D, Singh Y, Sharma AK. A simple and efficient agrobacterium-mediated procedure for transformation of tomato. J Biosci. 2009;34(3):423–33.van Eck J, Kirk DD, Walmsley AM. Tomato (Lycopersicum esculentum). Agrobacterium Protocols. 2006:459–74.Dan Y, Yan H, Munyikwa T, Dong J, Zhang Y, Armstrong CL. MicroTom—a high-throughput model transformation system for functional genomics. Plant Cell Rep. 2006;25(5):432–41.Pearce G, Strydom D, Johnson S, Ryan CA. A polypeptide from tomato leaves induces wound-inducible proteinase inhibitor proteins. Science. 1991;253(5022):895–9.Farmer EE, Ryan CA. Interplant communication: airborne methyl jasmonate induces synthesis of proteinase inhibitors in plant leaves. Proc Natl Acad Sci. 1990;87(19):7713–6.Bosch M, Wright LP, Gershenzon J, Wasternack C, Hause B, Schaller A, Stintzi A. Jasmonic acid and its precursor 12-oxophytodienoic acid control different aspects of constitutive and induced herbivore defenses in tomato. Plant Physiol. 2014;166(1):396–410.Christensen SA, Nemchenko A, Borrego E, Murray I, Sobhy IS, Bosak L, DeBlasio S, Erb M, Robert CA, Vaughn KA. The maize lipoxygenase, ZmLOX10, mediates green leaf volatile, jasmonate and herbivore-induced plant volatile production for defense against insect attack. Plant J. 2013;74(1):59–73.Boughton AJ, Hoover K, Felton GW. Methyl jasmonate application induces increased densities of glandular trichomes on tomato, Lycopersicon esculentum. J Chem Ecol. 2005;31(9):2211–6.Li L, Zhao Y, McCaig BC, Wingerd BA, Wang J, Whalon ME, Pichersky E, Howe GA. The tomato homolog of CORONATINE-INSENSITIVE1 is required for the maternal control of seed maturation, jasmonate-signaled defense responses, and glandular trichome development. Plant Cell. 2004;16(1):126–43.Peiffer M, Tooker JF, Luthe DS, Felton GW. Plants on early alert: glandular trichomes as sensors for insect herbivores. New Phytol. 2009;184(3):644–56.Bryant J, Green TR, Gurusaddaiah T, Ryan CA. Proteinase inhibitor II from potatoes: isolation and characterization of its protomer components. Biochemistry. 1976;15(16):3418–24.Johnson R, Narvaez J, An G, Ryan C. Expression of proteinase inhibitors I and II in transgenic tobacco plants: effects on natural defense against Manduca sexta larvae. Proc Natl Acad Sci. 1989;86(24):9871–5.Klopfenstein NB, Allen KK, Avila FJ, Heuchelin SA, Martinez J, Carman RC, Hall RB, Hart ER, McNabb HS. Proteinase inhibitor II gene in transgenic poplar: chemical and biological assays. Biomass Bioenergy. 1997;12(4):299–311.Dicke M, Takabayashi J, Posthumus MA, Schütte C, Krips OE. Plant—Phytoseiid interactions mediated by herbivore-induced plant volatiles: variation in production of cues and in responses of predatory mites. Exp Appl Acarol. 1998;22(6):311–33.Turlings T, Loughrin JH, Mccall PJ, Röse U, Lewis WJ, Tumlinson JH. How caterpillar-damaged plants protect themselves by attracting parasitic wasps. Proc Natl Acad Sci. 1995;92(10):4169–74.Levin DA. The role of trichomes in plant defense. Q Rev Biol. 1973;48(1, Part 1):3–15.Traw BM, Dawson TE. Differential induction of trichomes by three herbivores of black mustard. Oecologia. 2002;131(4):526–32.Handley R, Ekbom B, Ågren J. Variation in trichome density and resistance against a specialist insect herbivore in natural populations of Arabidopsis thaliana. Ecological Entomology. 2005;30(3):284–92.Valverde P, Fornoni J, NÚÑez-Farfán J. Defensive role of leaf trichomes in resistance to herbivorous insects in Datura stramonium. J Evol Biol. 2001;14(3):424–32.Elle E, Hare J. Environmentally induced variation in floral traits affects the mating system in Datura wrightii. Funct Ecol. 2002;16(1):79–88.Agrawal AA. Benefits and costs of induced plant defense for Lepidium virginicum (Brassicaceae). Ecology. 2000;81(7):1804–13.Dalin P, Björkman C. Adult beetle grazing induces willow trichome defence against subsequent larval feeding. Oecologia. 2003;134(1):112–8.Campos MR, Biondi A, Adiga A, Guedes RN, Desneux N. From the western Palaearctic region to beyond: Tuta absoluta 10 years after invading Europe. J Pest Sci. 2017:1–10.Desneux N, Wajnberg E, Wyckhuys KA, Burgio G, Arpaia S, Narváez-Vasquez CA, González-Cabrera J, Ruescas DC, Tabone E, Frandon J. Biological invasion of European tomato crops by Tuta absoluta: ecology, geographic expansion and prospects for biological control. J Pest Sci. 2010;83(3):197–215.Urbaneja A, Montón H, Mollá O. Suitability of the tomato borer Tuta absoluta as prey for Macrolophus pygmaeus and Nesidiocoris tenuis. J Appl Entomol. 2009;133(4):292–6.Pérez-Hedo M, Urbaneja A. Prospects for predatory mirid bugs as biocontrol agents of aphids in sweet peppers. J Pest Sci. 2015;88(1):65–73.Hewitt E. The composition of the nutrient solution. Sand and water culture methods used in the study of plant Nutrition. 1966:187–246.Karimi M, Inzé D, Depicker A. GATEWAY™ vectors for agrobacterium-mediated plant transformation. Trends Plant Sci. 2002;7(5):193–5.Martín-Trillo M, Grandío EG, Serra F, Marcel F, Rodríguez-Buey ML, Schmitz G, Theres K, Bendahmane A, Dopazo H, Cubas P. Role of tomato BRANCHED1-like genes in the control of shoot branching. Plant J. 2011;67(4):701–14.Vargas C. Observations on the bionomics and natural enemies of the tomato moth, Gnorimoschema absoluta (Meyrick)(Lep. Gelechiidae). Idesia. 1970;1:75–110.Mollá O, Biondi A, Alonso-Valiente M, Urbaneja A. A comparative life history study of two mirid bugs preying on Tuta absoluta and Ephestia kuehniella eggs on tomato crops: implications for biological control. BioControl. 2014;59(2):175–83.Abbot C. Solar variation and the weather. Science (New York, NY). 1925;62(1605):307.Bradford MM. A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein-dye binding. Anal Biochem. 1976;72(1–2):248–54.Bouagga S, Urbaneja A, Rambla JL, Granell A, Pérez-Hedo M. Orius laevigatus strengthens its role as a biological control agent by inducing plant defenses. J Pest Sci. 2017:1–10.Hilder VA, Gatehouse AM, Sheerman SE, Barker RF, Boulter D. A novel mechanism of insect resistance engineered into tobacco. Nature. 1987;330(6144):160–3.Saikia K, Kalita J, Saikia PK. Biology and life cycle generations of common crow–Euploea core core Cramer (Lepidoptera: Danainae) on Hemidesmus indica host plant. Int J NeBIO. 2010;1(3):28–37.Srinivasan A, Giri AP, Gupta VS. Structural and functional diversities in lepidopteran serine proteases. Cellular & molecular biology letters. 2006;11(1):132.Tamhane VA, Chougule NP, Giri AP, Dixit AR, Sainani MN, Gupta VS. In vivo and in vitro effect of Capsicum annum proteinase inhibitors on Helicoverpa armigera gut proteinases. Biochimica et Biophysica Acta (BBA)-General Subjects. 2005;1722(2):156–67.Telang M, Srinivasan A, Patankar A, Harsulkar A, Joshi V, Damle A, Deshpande V, Sainani M, Ranjekar P, Gupta G. Bitter gourd proteinase inhibitors: potential growth inhibitors of Helicoverpa armigera and Spodoptera litura. Phytochemistry. 2003;63(6):643–52.Damle MS, Giri AP, Sainani MN, Gupta VS. Higher accumulation of proteinase inhibitors in flowers than leaves and fruits as a possible basis for differential feeding preference of Helicoverpa armigera on tomato (Lycopersicon esculentum mill, cv. Dhanashree). Phytochemistry. 2005;66(22):2659–67.De Leo F, Bonadé-Bottino MA, Ceci LR, Gallerani R, Jouanin L. Opposite effects on spodoptera littoralis larvae of high expression level of a trypsin proteinase inhibitor in transgenic plants. Plant Physiol. 1998;118(3):997–1004.Rahbé Y, Ferrasson E, Rabesona H, Quillien L. Toxicity to the pea aphid Acyrthosiphon pisum of anti-chymotrypsin isoforms and fragments of Bowman–Birk protease inhibitors from pea seeds. Insect Biochem Mol Biol. 2003;33(3):299–306.Luo M, Ding L-W, Ge Z-J, Wang Z-Y, Hu B-L, Yang X-B, Sun Q-Y, Xu Z-F. The characterization of SaPIN2b, a plant trichome-localized proteinase inhibitor from Solanum americanum. Int J Mol Sci. 2012;13(11):15162–76.Dalin P, Ågren J, Björkman C, Huttunen P, Kärkkäinen K. Leaf trichome formation and plant resistance to herbivory. In: Dordrecht SA, editor. Induced plant resistance to herbivory. Netherlands: Springer; 2008. p. 89–105.Gonzáles WL, Negritto MA, Suárez LH, Gianoli E. Induction of glandular and non-glandular trichomes by damage in leaves of Madia sativa under contrasting water regimes. Acta Oecol. 2008;33(1):128–32.Luo M, Wang Z, Li H, Xia K-F, Cai Y, Xu Z-F. Overexpression of a weed (Solanum americanum) proteinase inhibitor in transgenic tobacco results in increased glandular trichome density and enhanced resistance to Helicoverpa armigera and Spodoptera litura. Int J Mol Sci. 2009;10(4):1896–910.Björkman C, Dalin P, Ahrné K. Leaf trichome responses to herbivory in willows: induction, relaxation and costs. New Phytol. 2008;179(1):176–84.Duffey S. Plant glandular trichomes: their partial role in defence against insects. Insects and the plant surface. London: Edward Arnold; 1986. p. 151–72.James DG. Further field evaluation of synthetic herbivore-induced plan volatiles as attractants for beneficial insects. J Chem Ecol. 2005;31(3):481–95.Naselli M, Zappalà L, Gugliuzzo A, Garzia GT, Biondi A, Rapisarda C, Cincotta F, Condurso C, Verzera A, Siscaro G. Olfactory response of the zoophytophagous mirid Nesidiocoris tenuis to tomato and alternative host plants. Arthropod Plant Interact. 2017;11(2):121–31.Tholl D. Biosynthesis and biological functions of terpenoids in plants. Advances in Biochemical Engineering and Biotechnology. 2015;148:63-106.Lange BM, Rujan T, Martin W, Croteau R. Isoprenoid biosynthesis: the evolution of two ancient and distinct pathways across genomes. Proc Natl Acad Sci. 2000;97(24):13172–7.Dudareva N, Klempien A, Muhlemann JK, Kaplan I. Biosynthesis, function and metabolic engineering of plant volatile organic compounds. New Phytol. 2013;198(1):16–32.Razal RA, Ellis S, Singh S, Lewis NG, Towers GHN. Nitrogen recycling in phenylpropanoid metabolism. Phytochemistry. 1996;41(1):31–5.Effmert U, Große J, Röse US, Ehrig F, Kägi R, Piechulla B. Volatile composition, emission pattern, and localization of floral scent emission in Mirabilis jalapa (Nyctaginaceae). Am J Bot. 2005;92(1):2–12.Guterman I, Masci T, Chen X, Negre F, Pichersky E, Dudareva N, Weiss D, Vainstein A. Generation of phenylpropanoid pathway-derived volatiles in transgenic plants: rose alcohol acetyltransferase produces phenylethyl acetate and benzyl acetate in petunia flowers. Plant Mol Biol. 2006;60(4):555–63.Vogel JT, Tan B-C, McCarty DR, Klee HJ. The carotenoid cleavage dioxygenase 1 enzyme has broad substrate specificity, cleaving multiple carotenoids at two different bond positions. J Biol Chem. 2008;283(17):11364–73.Colquhoun TA, Kim JY, Wedde AE, Levin LA, Schmitt KC, Schuurink RC, Clark DG. PhMYB4 fine-tunes the floral volatile signature of petunia×hybrida through PhC4H. J Exp Bot. 2011;62(3):1133–43.Kolosova N, Gorenstein N, Kish CM, Dudareva N. Regulation of circadian methyl benzoate emission in diurnally and nocturnally emitting plants. Plant Cell. 2001;13(10):2333–47.Maeda H, Shasany AK, Schnepp J, Orlova I, Taguchi G, Cooper BR, Rhodes D, Pichersky E, Dudareva N. RNAi suppression of arogenate dehydratase1 reveals that phenylalanine is synthesized predominantly via the arogenate pathway in petunia petals. Plant Cell. 2010;22(3):832–49.Lerdau M, Gray D. Ecology and evolution of light-dependent and light-independent phytogenic volatile organic carbon. New Phytol. 2003;157(2):199–211.Martin DM, Gershenzon J, Bohlmann J. Induction of volatile terpene biosynthesis and diurnal emission by methyl jasmonate in foliage of Norway spruce. Plant Physiol. 2003;132(3):1586–99.van Doorn WG, Woltering EJ. Physiology and molecular biology of petal senescence. J Exp Bot. 2008;59(3):453–80

    Impact of volatile phenols and their precursors on wine quality and control measures of Brettanomyces/Dekkera yeasts

    Get PDF
    Volatile phenols are aromatic compounds and one of the key molecules responsible for olfactory defects in wine. The yeast genus Brettanomyces is the only major microorganism that has the ability to covert hydroxycinnamic acids into important levels of these compounds, especially 4-ethylphenol and 4-ethylguaiacol, in red wine. When 4-ethylphenols reach concentrations greater than the sensory threshold, all wine’s organoleptic characteristics might be influenced or damaged. The aim of this literature review is to provide a better understanding of the physicochemical, biochemical, and metabolic factors that are related to the levels of p-coumaric acid and volatile phenols in wine. Then, this work summarizes the different methods used for controlling the presence of Brettanomyces in wine and the production of ethylphenols

    Two euAGAMOUS genes control C-function in Medicago truncatula

    Get PDF
    [EN] C-function MADS-box transcription factors belong to the AGAMOUS (AG) lineage and specify both stamen and carpel identity and floral meristem determinacy. In core eudicots, the AG lineage is further divided into two branches, the euAG and PLE lineages. Functional analyses across flowering plants strongly support the idea that duplicated AG lineage genes have different degrees of subfunctionalization of the C-function. The legume Medicago truncatula contains three C-lineage genes in its genome: two euAG genes (MtAGa and MtAGb) and one PLENA-like gene (MtSHP). This species is therefore a good experimental system to study the effects of gene duplication within the AG subfamily. We have studied the respective functions of each euAG genes in M. truncatula employing expression analyses and reverse genetic approaches. Our results show that the M. truncatula euAG- and PLENA-like genes are an example of subfunctionalization as a result of a change in expression pattern. MtAGa and MtAGb are the only genes showing a full C-function activity, concomitant with their ancestral expression profile, early in the floral meristem, and in the third and fourth floral whorls during floral development. In contrast, MtSHP expression appears late during floral development suggesting it does not contribute significantly to the C-function. Furthermore, the redundant MtAGa and MtAGb paralogs have been retained which provides the overall dosage required to specify the C-function in M. truncatula.This work was funded by grants BIO2009-08134 and BIO2012-39849-C02-01 from the Spanish Ministry of Economy and Competitiveness and the Ramon y Cajal Program (RYC-2007-00627 to CGM). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.Serwatowska, J.; Roque Mesa, EM.; Gómez Mena, MC.; Constantin, GD.; Wen, J.; Mysore, KS.; Lund, OS.... (2014). Two euAGAMOUS genes control C-function in Medicago truncatula. PLoS ONE. 9(8):103770-1-103770-12. https://doi.org/10.1371/journal.pone.0103770S103770-1103770-1298Prunet, N., & Jack, T. P. (2013). Flower Development in Arabidopsis: There Is More to It Than Learning Your ABCs. Flower Development, 3-33. doi:10.1007/978-1-4614-9408-9_1Causier, B., Schwarz-Sommer, Z., & Davies, B. (2010). Floral organ identity: 20 years of ABCs. Seminars in Cell & Developmental Biology, 21(1), 73-79. doi:10.1016/j.semcdb.2009.10.005Irish, V. F. (2010). The flowering of Arabidopsis flower development. The Plant Journal, 61(6), 1014-1028. doi:10.1111/j.1365-313x.2009.04065.xHeijmans, K., Morel, P., & Vandenbussche, M. (2012). MADS-box Genes and Floral Development: the Dark Side. Journal of Experimental Botany, 63(15), 5397-5404. doi:10.1093/jxb/ers233Bowman, J. L., Smyth, D. R., & Meyerowitz, E. M. (1989). Genes directing flower development in Arabidopsis. The Plant Cell, 1(1), 37-52. doi:10.1105/tpc.1.1.37Yanofsky, M. F., Ma, H., Bowman, J. L., Drews, G. N., Feldmann, K. A., & Meyerowitz, E. M. (1990). The protein encoded by the Arabidopsis homeotic gene agamous resembles transcription factors. Nature, 346(6279), 35-39. doi:10.1038/346035a0Bradley, D., Carpenter, R., Sommer, H., Hartley, N., & Coen, E. (1993). Complementary floral homeotic phenotypes result from opposite orientations of a transposon at the plena locus of antirrhinum. Cell, 72(1), 85-95. doi:10.1016/0092-8674(93)90052-rPinyopich, A., Ditta, G. S., Savidge, B., Liljegren, S. J., Baumann, E., Wisman, E., & Yanofsky, M. F. (2003). Assessing the redundancy of MADS-box genes during carpel and ovule development. Nature, 424(6944), 85-88. doi:10.1038/nature01741Liljegren, S. J., Ditta, G. S., Eshed, Y., Savidge, B., Bowman, J. L., & Yanofsky, M. F. (2000). SHATTERPROOF MADS-box genes control seed dispersal in Arabidopsis. Nature, 404(6779), 766-770. doi:10.1038/35008089Davies, B., Motte, P., Keck, E., Saedler, H., Sommer, H., & Schwarz-Sommer, Z. (1999). PLENA and FARINELLI: redundancy and regulatory interactions between two Antirrhinum MADS-box factors controlling flower development. The EMBO Journal, 18(14), 4023-4034. doi:10.1093/emboj/18.14.4023Kramer, E. M., Jaramillo, M. A., & Di Stilio, V. S. (2004). Patterns of Gene Duplication and Functional Evolution During the Diversification of the AGAMOUS Subfamily of MADS Box Genes in Angiosperms. Genetics, 166(2), 1011-1023. doi:10.1534/genetics.166.2.1011Becker, A. (2003). The major clades of MADS-box genes and their role in the development and evolution of flowering plants. Molecular Phylogenetics and Evolution, 29(3), 464-489. doi:10.1016/s1055-7903(03)00207-0Irish, V. F. (2003). The evolution of floral homeotic gene function. BioEssays, 25(7), 637-646. doi:10.1002/bies.10292Zahn, L. M., Leebens-Mack, J. H., Arrington, J. M., Hu, Y., Landherr, L. L., dePamphilis, C. W., … Ma, H. (2006). Conservation and divergence in the AGAMOUS subfamily of MADS-box genes: evidence of independent sub- and neofunctionalization events. Evolution Development, 8(1), 30-45. doi:10.1111/j.1525-142x.2006.05073.xFerrandiz, C. (2000). Negative Regulation of the SHATTERPROOF Genes by FRUITFULL During Arabidopsis Fruit Development. Science, 289(5478), 436-438. doi:10.1126/science.289.5478.436Ma, H., Yanofsky, M. F., & Meyerowitz, E. M. (1991). AGL1-AGL6, an Arabidopsis gene family with similarity to floral homeotic and transcription factor genes. Genes & Development, 5(3), 484-495. doi:10.1101/gad.5.3.484Savidge, B., Rounsley, S. D., & Yanofsky, M. F. (1995). Temporal relationship between the transcription of two Arabidopsis MADS box genes and the floral organ identity genes. The Plant Cell, 7(6), 721-733. doi:10.1105/tpc.7.6.721Colombo, M., Brambilla, V., Marcheselli, R., Caporali, E., Kater, M. M., & Colombo, L. (2010). A new role for the SHATTERPROOF genes during Arabidopsis gynoecium development. Developmental Biology, 337(2), 294-302. doi:10.1016/j.ydbio.2009.10.043Fourquin, C., & Ferrándiz, C. (2012). Functional analyses of AGAMOUS family members in Nicotiana benthamiana clarify the evolution of early and late roles of C-function genes in eudicots. The Plant Journal, 71(6), 990-1001. doi:10.1111/j.1365-313x.2012.05046.xKapoor, M., Tsuda, S., Tanaka, Y., Mayama, T., Okuyama, Y., Tsuchimoto, S., & Takatsuji, H. (2002). Role of petuniapMADS3in determination of floral organ and meristem identity, as revealed by its loss of function. The Plant Journal, 32(1), 115-127. doi:10.1046/j.1365-313x.2002.01402.xPan, I. L., McQuinn, R., Giovannoni, J. J., & Irish, V. F. (2010). Functional diversification of AGAMOUS lineage genes in regulating tomato flower and fruit development. Journal of Experimental Botany, 61(6), 1795-1806. doi:10.1093/jxb/erq046Pnueli, L., Hareven, D., Rounsley, S. D., Yanofsky, M. F., & Lifschitz, E. (1994). Isolation of the tomato AGAMOUS gene TAG1 and analysis of its homeotic role in transgenic plants. The Plant Cell, 6(2), 163-173. doi:10.1105/tpc.6.2.163Dreni, L., & Kater, M. M. (2013). MADSreloaded: evolution of theAGAMOUSsubfamily genes. New Phytologist, 201(3), 717-732. doi:10.1111/nph.12555Brunner, A. M. (2000). Plant Molecular Biology, 44(5), 619-634. doi:10.1023/a:1026550205851Perl-Treves, R., Kahana, A., Rosenman, N., Xiang, Y., & Silberstein, L. (1998). Expression of Multiple AGAMOUS-Like Genes in Male and Female Flowers of Cucumber (Cucumis sativus L.). Plant and Cell Physiology, 39(7), 701-710. doi:10.1093/oxfordjournals.pcp.a029424Yu, D., Kotilainen, M., Pöllänen, E., Mehto, M., Elomaa, P., Helariutta, Y., … Teeri, T. H. (1999). Organ identity genes and modified patterns of flower development in Gerbera hybrida (Asteraceae). The Plant Journal, 17(1), 51-62. doi:10.1046/j.1365-313x.1999.00351.xDong, Z., Zhao, Z., Liu, C., Luo, J., Yang, J., Huang, W., … Luo, D. (2005). Floral Patterning in Lotus japonicus. Plant Physiology, 137(4), 1272-1282. doi:10.1104/pp.104.054288Hofer, J. M., & Noel Ellis, T. (2014). Developmental specialisations in the legume family. Current Opinion in Plant Biology, 17, 153-158. doi:10.1016/j.pbi.2013.11.014Fourquin, C., del Cerro, C., Victoria, F. C., Vialette-Guiraud, A., de Oliveira, A. C., & Ferrándiz, C. (2013). A Change in SHATTERPROOF Protein Lies at the Origin of a Fruit Morphological Novelty and a New Strategy for Seed Dispersal in Medicago Genus. Plant Physiology, 162(2), 907-917. doi:10.1104/pp.113.217570Hewitt EJ (1966) Sand and Water Culture Methods Used in the Study of Plant Nutrition. Farnham Royal, UK: Commonwealth Agricultural Bureau.Cheng, X., Wang, M., Lee, H.-K., Tadege, M., Ratet, P., Udvardi, M., … Wen, J. (2013). An efficient reverse genetics platform in the model legumeMedicago truncatula. New Phytologist, 201(3), 1065-1076. doi:10.1111/nph.12575D’ Erfurth, I., Cosson, V., Eschstruth, A., Lucas, H., Kondorosi, A., & Ratet, P. (2003). Efficient transposition of theTnt1tobacco retrotransposon in the model legumeMedicago truncatula. The Plant Journal, 34(1), 95-106. doi:10.1046/j.1365-313x.2003.01701.xTadege, M., Ratet, P., & Mysore, K. S. (2005). Insertional mutagenesis: a Swiss Army knife for functional genomics of Medicago truncatula. Trends in Plant Science, 10(5), 229-235. doi:10.1016/j.tplants.2005.03.009Tadege, M., Wen, J., He, J., Tu, H., Kwak, Y., Eschstruth, A., … Mysore, K. S. (2008). Large-scale insertional mutagenesis using the Tnt1 retrotransposon in the model legume Medicago truncatula. The Plant Journal, 54(2), 335-347. doi:10.1111/j.1365-313x.2008.03418.xCheng, X., Wen, J., Tadege, M., Ratet, P., & Mysore, K. S. (2010). Reverse Genetics in Medicago truncatula Using Tnt1 Insertion Mutants. Plant Reverse Genetics, 179-190. doi:10.1007/978-1-60761-682-5_13Benlloch, R., d’ Erfurth, I., Ferrandiz, C., Cosson, V., Beltrán, J. P., Cañas, L. A., … Ratet, P. (2006). Isolation of mtpim Proves Tnt1 a Useful Reverse Genetics Tool in Medicago truncatula and Uncovers New Aspects of AP1-Like Functions in Legumes. Plant Physiology, 142(3), 972-983. doi:10.1104/pp.106.083543Larkin, M. A., Blackshields, G., Brown, N. P., Chenna, R., McGettigan, P. A., McWilliam, H., … Higgins, D. G. (2007). Clustal W and Clustal X version 2.0. Bioinformatics, 23(21), 2947-2948. doi:10.1093/bioinformatics/btm404Altschul, S. (1997). Gapped BLAST and PSI-BLAST: a new generation of protein database search programs. Nucleic Acids Research, 25(17), 3389-3402. doi:10.1093/nar/25.17.3389Tamura, K., Dudley, J., Nei, M., & Kumar, S. (2007). MEGA4: Molecular Evolutionary Genetics Analysis (MEGA) Software Version 4.0. Molecular Biology and Evolution, 24(8), 1596-1599. doi:10.1093/molbev/msm092Dellaporta, S. L., Wood, J., & Hicks, J. B. (1983). A plant DNA minipreparation: Version II. Plant Molecular Biology Reporter, 1(4), 19-21. doi:10.1007/bf02712670Schmittgen, T. D., & Livak, K. J. (2008). Analyzing real-time PCR data by the comparative CT method. Nature Protocols, 3(6), 1101-1108. doi:10.1038/nprot.2008.73Constantin, G. D., Krath, B. N., MacFarlane, S. A., Nicolaisen, M., Elisabeth Johansen, I., & Lund, O. S. (2004). Virus-induced gene silencing as a tool for functional genomics in a legume species. The Plant Journal, 40(4), 622-631. doi:10.1111/j.1365-313x.2004.02233.xWesley, S. V., Helliwell, C. A., Smith, N. A., Wang, M., Rouse, D. T., Liu, Q., … Waterhouse, P. M. (2001). Construct design for efficient, effective and high-throughput gene silencing in plants. The Plant Journal, 27(6), 581-590. doi:10.1046/j.1365-313x.2001.01105.xGuerineau F, Mullineaux P (1993) Plant transformation and expression vectors. In: Croy R, editor. Plant Molecular Biology. Oxford, UK: Bios Scientific Publishers, Academic Press. pp. 121–147.Clough, S. J., & Bent, A. F. (1998). Floral dip: a simplified method forAgrobacterium-mediated transformation ofArabidopsis thaliana. The Plant Journal, 16(6), 735-743. doi:10.1046/j.1365-313x.1998.00343.xBenlloch, R., Roque, E., Ferrándiz, C., Cosson, V., Caballero, T., Penmetsa, R. V., … Madueño, F. (2009). Analysis of B function in legumes: PISTILLATA proteins do not require the PI motif for floral organ development inMedicago truncatula. The Plant Journal, 60(1), 102-111. doi:10.1111/j.1365-313x.2009.03939.xRoque, E., Serwatowska, J., Cruz Rochina, M., Wen, J., Mysore, K. S., Yenush, L., … Cañas, L. A. (2012). Functional specialization of duplicated AP3-like genes inMedicago truncatula. The Plant Journal, 73(4), 663-675. doi:10.1111/tpj.12068Flanagan, C. A., Hu, Y., & Ma, H. (1996). Specific expression of the AGL1 MADS-box gene suggests regulatory functions in Arabidopsis gynoecium and ovule development. The Plant Journal, 10(2), 343-353. doi:10.1046/j.1365-313x.1996.10020343.xSieburth, L. E., & Meyerowitz, E. M. (1997). Molecular dissection of the AGAMOUS control region shows that cis elements for spatial regulation are located intragenically. The Plant Cell, 9(3), 355-365. doi:10.1105/tpc.9.3.355Busch, M. A. (1999). Activation of a Floral Homeotic Gene in Arabidopsis. Science, 285(5427), 585-587. doi:10.1126/science.285.5427.585Moyroud, E., Minguet, E. G., Ott, F., Yant, L., Posé, D., Monniaux, M., … Parcy, F. (2011). Prediction of Regulatory Interactions from Genome Sequences Using a Biophysical Model for the Arabidopsis LEAFY Transcription Factor. The Plant Cell, 23(4), 1293-1306. doi:10.1105/tpc.111.083329Grønlund, M., Constantin, G., Piednoir, E., Kovacev, J., Johansen, I. E., & Lund, O. S. (2008). Virus-induced gene silencing in Medicago truncatula and Lathyrus odorata. Virus Research, 135(2), 345-349. doi:10.1016/j.virusres.2008.04.005Mandel, M. A., Bowman, J. L., Kempin, S. A., Ma, H., Meyerowitz, E. M., & Yanofsky, M. F. (1992). Manipulation of flower structure in transgenic tobacco. Cell, 71(1), 133-143. doi:10.1016/0092-8674(92)90272-eMizukami, Y., & Ma, H. (1992). Ectopic expression of the floral homeotic gene AGAMOUS in transgenic Arabidopsis plants alters floral organ identity. Cell, 71(1), 119-131. doi:10.1016/0092-8674(92)90271-dCannon, S. B., Sterck, L., Rombauts, S., Sato, S., Cheung, F., Gouzy, J., … Young, N. D. (2006). Legume genome evolution viewed through the Medicago truncatula and Lotus japonicus genomes. Proceedings of the National Academy of Sciences, 103(40), 14959-14964. doi:10.1073/pnas.0603228103Young, N. D., & Bharti, A. K. (2012). Genome-Enabled Insights into Legume Biology. Annual Review of Plant Biology, 63(1), 283-305. doi:10.1146/annurev-arplant-042110-103754Jager, M. (2003). MADS-Box Genes in Ginkgo biloba and the Evolution of the AGAMOUS Family. Molecular Biology and Evolution, 20(5), 842-854. doi:10.1093/molbev/msg089Johansen, B., Pedersen, L. B., Skipper, M., & Frederiksen, S. (2002). MADS-box gene evolution—structure and transcription patterns. Molecular Phylogenetics and Evolution, 23(3), 458-480. doi:10.1016/s1055-7903(02)00032-5Rutledge, R., Regan, S., Nicolas, O., Fobert, P., Côté, C., Bosnich, W., … Stewart, D. (1998). Characterization of an AGAMOUS homologue from the conifer black spruce ( Picea mariana ) that produces floral homeotic conversions when expressed in Arabidopsis. The Plant Journal, 15(5), 625-634. doi:10.1046/j.1365-313x.1998.00250.xParcy, F., Nilsson, O., Busch, M. A., Lee, I., & Weigel, D. (1998). A genetic framework for floral patterning. Nature, 395(6702), 561-566. doi:10.1038/26903Causier, B., Bradley, D., Cook, H., & Davies, B. (2009). Conserved intragenic elements were critical for the evolution of the floral C-function. The Plant Journal, 58(1), 41-52. doi:10.1111/j.1365-313x.2008.03759.xAiroldi, C. A., & Davies, B. (2012). Gene Duplication and the Evolution of Plant MADS-box Transcription Factors. Journal of Genetics and Genomics, 39(4), 157-165. doi:10.1016/j.jgg.2012.02.008Giménez, E., Pineda, B., Capel, J., Antón, M. T., Atarés, A., Pérez-Martín, F., … Lozano, R. (2010). Functional Analysis of the Arlequin Mutant Corroborates the Essential Role of the ARLEQUIN/TAGL1 Gene during Reproductive Development of Tomato. PLoS ONE, 5(12), e14427. doi:10.1371/journal.pone.0014427Kater, M. M., Colombo, L., Franken, J., Busscher, M., Masiero, S., Van Lookeren Campagne, M. M., & Angenent, G. C. (1998). Multiple AGAMOUS Homologs from Cucumber and Petunia Differ in Their Ability to Induce Reproductive Organ Fate. The Plant Cell, 10(2), 171-182. doi:10.1105/tpc.10.2.171Tsuchimoto, S., van der Krol, A. R., & Chua, N. H. (1993). Ectopic expression of pMADS3 in transgenic petunia phenocopies the petunia blind mutant. The Plant Cell, 5(8), 843-853. doi:10.1105/tpc.5.8.843Airoldi, C. A., Bergonzi, S., & Davies, B. (2010). Single amino acid change alters the ability to specify male or female organ identity. Proceedings of the National Academy of Sciences, 107(44), 18898-18902. doi:10.1073/pnas.1009050107Causier, B., Castillo, R., Zhou, J., Ingram, R., Xue, Y., Schwarz-Sommer, Z., & Davies, B. (2005). Evolution in Action: Following Function in Duplicated Floral Homeotic Genes. Current Biology, 15(16), 1508-1512. doi:10.1016/j.cub.2005.07.063Birchler, J. A., & Veitia, R. A. (2007). The Gene Balance Hypothesis: From Classical Genetics to Modern Genomics. The Plant Cell, 19(2), 395-402. doi:10.1105/tpc.106.049338Birchler, J. A., & Veitia, R. A. (2009). The gene balance hypothesis: implications for gene regulation, quantitative traits and evolution. New Phytologist, 186(1), 54-62. doi:10.1111/j.1469-8137.2009.03087.xEdger, P. P., & Pires, J. C. (2009). Gene and genome duplications: the impact of dosage-sensitivity on the fate of nuclear genes. Chromosome Research, 17(5), 699-717. doi:10.1007/s10577-009-9055-9Freeling, M. (2006). Gene-balanced duplications, like tetraploidy, provide predictable drive to increase morphological complexity. Genome Research, 16(7), 805-814. doi:10.1101/gr.368140

    Design for Mobile Mental Health:An Exploratory Review

    Get PDF
    A large number of mobile mental health apps are available to the public but current knowledge about requirements of designing such solutions is scarce, especially from sociotechnical and user centred points of view. Due to the significant role of mobile apps in the mental health service models, identifying the design requirements of mobile mental health solutions is crucial. Some of those requirements have been addressed individually in the literature, but there are few research studies that show a comprehensive picture of this domain. This exploratory review aims to facilitate such holistic understanding. The main search keywords of the review were identified in a cross-disciplinary requirements workshop. The search was started by finding some core references in the healthcare databases. A wider range of references then has been explored using a snowball method. Findings showed that there is a good understanding of individual design requirements in current literature but there are few examples of implementing a combination of different design requirements in real world products. The design processes specifically developed for mobile mental health apps are also rare. Most studies on operational mobile mental health apps address major mental health issues while prevention and wellbeing areas are underdeveloped. In conclusion, the main recommendations for designing future mobile mental health solutions include: moving towards sociotechnical and open design strategies, understanding and creating shared value, recognizing all dimensions of efficacy, bridging design and medical research and development, and considering an ecosystem perspective

    A foodomics approach: CE-MS for comparative metabolomics of colon cancer cells treated with dietary polyphenols

    No full text
    The potential of capillary electrophoresis-mass spectrometry (CE-MS) for metabolomics is demonstrated through the analysis of metabolites from human HT29 colon cancer cells treated and non-treated with dietary polyphenols. Prior to CE-MS analysis, four different metabolite purification strategies are investigated. Namely, the results obtained after methanol deproteinization, ultrafiltration, and two solid-phase extraction methods using C18 and polymer-based cartridges are described. These generic methods can have broad applications to analyze metabolites in a large variety of matrices and fields, including the new Foodomics area.This work was supported by AGL2008-05108-C03-01 (Ministerio de Ciencia e InnovaciĂłn, Spain) and CSD2007-00063 FUN-C-FOOD projects (Programa CONSOLIDER, Ministerio de Educacion y Ciencia, Spain). MC thanks the Council of Higher Education, Turkey, for his grant. CI thanks Ministerio de Educacion y Ciencia, Spain, for her FPI grant.Peer reviewe
    corecore