Abstract
Pollen tube growth is localized at the apex and displays oscillatory dynamics. It is thought that a balance between intracellular turgor pressure (hydrostatic pressure, reflected by the cell volume) and cell wall loosening is a critical factor driving pollen tube growth. We previously demonstrated that water flows freely into and out of the pollen tube apical region dependent on the extracellular osmotic potential, that cell volume changes reflect changes in the intracellular pressure, and that cell volume changes differentially induce, increases or decreases in specific phospholipid signals. This article shows that manipulation of the extracellular osmotic potential rapidly induces modulations in pollen tube growth rate frequencies, demonstrating that changes in the intracellular pressure are sufficient to reset the pollen tube growth oscillator. This indicates a direct link between intracellular hydrostatic pressure and pollen tube growth. Altering hydrodynamic flow through the pollen tube by replacing extracellular H2O with 2H2O adversely affects both cell volume and growth rate oscillations and induces aberrant morphologies. Normal growth and cell morphology are rescued by replacing 2H2O with H2O. Further studies revealed that the cell volume oscillates in the pollen tube apical region. These cell volume oscillations were not from changes in cell shape at the tip and were detectable up to 30 μm distal to the tip (the longest length measured). Cell volume in the apical region oscillates with the same frequency as growth rate oscillations but surprisingly the cycles are phase-shifted by 180°. Raman microscopy yields evidence that hydrodynamic flow out of the apex may be part of the biomechanics that drive cellular expansion. The combined results suggest that hydrodynamic loading/unloading in the apical region induces cell volume oscillations and has a role in driving cell elongation and pollen tube growth.
Similar content being viewed by others
References
Zonia, L. and Munnik T. (2004) Osmotically induced cell swelling versus cell shrinking elicits specific changes in phospholipid signals in tobacco pollen tubes. Plant Physiol. 134, 813–823.
Holdaway-Clarke, T. L. and Hepler, P. K. (2003) Control of pollen tube growth: role of ion gradients and fluxes. New Phytol. 159, 539–563.
Lhuissier, F. G. P., de Ruijter, N. C. A., Sieberer, B. J., et al. (2001) Time course of cell biological events evoked in legume root hairs by Rhizobium Nod factors: state of the art. Ann. Bot. 87, 289–302.
Palanivelu, R. and Preuss, D. (2000) Pollen tube targeting and axon guidance: parallels in tip growth mechanisms. Trends Cell Biol. 10, 517–524.
Messerli, M. A. and Robinson, K. R. (2003) Ionic and osmotic disruptions of the lily pollen tube oscillator: testing proposed models. Planta 217, 147–157.
Higashiyama, T., Kuroiwa, H., Kawano, S. and Kuroiwa, T. (2000) Explosive discharge of pollen tube contents in Torenia fournieri. Plant Physiol. 122 11–13.
Hutt, M. T. and Luttge, U. (2002). Nonlinear dynamics as a tool for modeling in plant physiology. Plant Biol. 4, 281–297.
Parre, E. and Geitmann, A. (2005) Pectin and the role of the physical properties of the cell wall in pollen tube growth of Solanum chacoense. Planta 220, 582–592.
Bosch, M., Cheung, A. Y. and Hepler, P. K. (2005) Pectin methylesterase, a regulator of pollen tube growth. Plant Physiol. 138, 1334–1346.
Carpita, N. and Gibeaut, D. (1993) Structural models of primary cell walls in flowering plants: consistency of molecular structure with the physical properties of the wall during growth. Plant J. 3, 1–30.
Geitmann, A. and Parre, E. (2004) The local cytomechanical properties of growing pollen tubes correspond to the axial distribution of structural cellular elements. Sex. Plant Reprod. 17, 9–16.
Holdaway-Clarke, T. L., Weddle, N. M., Kim, S., et al. (2003) Effect of extracellular calcium, pH and borate on growth oscillations in Lilium formosanum pollen tubes. J. Exp. Bot. 54, 65–72.
Roy, S., Jauh, G. Y., Hepler, P. K. and Lord, E. M. (1998) Effects of Yariv phenylglycoside on cell wall assembly in the lily pollen tube. Planta 204, 450–458.
Zonia L., Cordeiro, S., Tupy J. and Feijo J. A. (2002) Oscillatory chloride efflux at the pollen tube apex has a role in growth and cell volume regulation and is targeted by inositol 3,4,5,6-tetrakisphosphate. Plant Cell 14, 2233–2249.
Wei, C. and Lintilhac, P. M. (2003) Loss of stability—a new model for stress relaxation in plant cell walls. J. Theor. Biol. 224 305–312.
Cosgrove, D. J. (1986). Biophysical control of plant cell growth. Annu. Rev. Plant Physiol. 37, 377–405.
Benkert, R., Obermeyer, G. and Bentrup, F.-W. (1997) The turgor pressure of growing lily pollen tubes. Protoplasma 198, 1–8.
Cardenas, L., Lovy-Wheeler, A., Wilsen, K. L. and Hepler, P. K. (2005) Actin polymerization promotes the reversal of streaming in the apex of pollen tubes. Cell Motil. Cytoskel. 61, 112–127.
Vervaeke, I., Delen, R., Wouters, J., et al. (2004) Semi in vivo pollen tube growth of Aechmea fasciata. Plant Cell Tissue Org. Cult. 76, 67–73.
Lin, Y. and Yang, Z. (1997) Inhibition of pollen tube elongation by microinjected anti-Rop 1Ps antibodies suggests a crucial role for Rho-Type GTPases in the control of tip growth. Plant Cell 9, 1647–1659.
Pierson, E. S., Miller, D. D., Callaham, D. A., et al., (1996) Tip-localized calcium entry fluctuates during pollen tube growth. Dev. Biol. 174, 160–173.
Malho R., Read, N. D., Trewavas, A. J. and Pais, M. S. (1995) Calcium-channel activity during pollen tube growth and reorientation. Plant Cell 7, 1173–1184.
Lazzaro, M. D., Donohue, J. M. and Soodavar, F. M. (2003) Disruption of cellulose synthesis by isoxaben causes tip swelling and disorganizes cortical microtubules in elongating conifer pollen tubes. Protoplasma 220, 201–207.
Vidali, L., McKenna, S. T. and Hepler, P. K. (2001) Actin polymerization is essential for pollen tube growth. Mol. Biol. Cell 12, 2534–2545.
Geitmann, A., Snowman, B. N., Emons, A. M. C. and Franklin-Tong, V. E. (2000) Alterations in the actin cytoskeleton of pollen tubes are induced by the self-incompatibility reaction in Papaver rhoeas. Plant Cell 12, 1239–1251.
Anderhag, P., Hepler, P. K. and Lazzaro, M. D. (2000) Microtubules and microfilaments are both responsible for pollen tube elongation in the conifer Picea abies (Norway spruce). Protoplasma 214, 141–157.
Monteiro D., Liu, Q. L., Lisboa, S., et al. (2005) Phosphoinositides and phosphatidic acid regulate pollen tube growth and reorientation through modulation of [Ca2+]cyt and membrane secretion. J. Exp. Bot. 56, 1665–1674.
Xu, J., Brearley, C. A., Lin, W. H., et al. (2005) A role of Arabidopsis inositol polyphosphate kinase, AtIPK2 alpha, in pollen germination and root growth. Plant Physiol. 137, 94–103.
Hunt, L., Otterhag, L., Lee, J. C., et al. (2004) Gene-specific expression and calcium activation of Arabidopsis thaliana phospholipase C isoforms. New Phytol. 162, 643–654.
Gupta, R., Ting, J. T. L., Sokolov, L. N., et al. (2002) A tumor suppressor homolog, AtPTEN1, is essential for pollen development in Arabidopsis. Plant Cell 14, 2495–2507.
Kost, B., Lemichez, E., Spielhofer, P., et al. (1999). Rac homologs and compartmentalized phosphatidylinositol 4,5-bisphosphate act in a common pathway to regulate polar pollen tube growth. J. Cell. Biol. 145, 317–330.
Malho, R. (1998) Role of 1,4,5-inositol trisphosphate-induced Ca2+ release in pollen tube orientation. Sex. Plant Reprod. 11, 231–235.
Franklin-Tong, V. E., Drøbak, B. K., Allan, A. C., et al. (1996) Growth of pollen tubes of Papaver rhoeas is regulated by a slow-moving calcium wave propagated by inositol 1,4,5-trisphosphate. Plant Cell 8, 1305–1321.
Zonia, L., and Munnik, T. Cracking the green paradigm: functional coding of phosphoinositide signals in plant stress responses. In Biology of Inositols and Phosphoinositides (Majumder A. L. and Biswas B., eds.). Springer Dordrecht, 2000, pp. 205–236.
de Groot, B. L., and Grubmüller, H. (2001) Water permeation across biological membranes: mechanism and dynamics of aquaporin-1 and GlpF. Science 294, 2353–2357.
Borgnia, M., Nielsen, S., Engel, A., and Agre, P. (1999) Cellular and molecular biology of the aquaporin water channels. Annu. Rev. Biochem. 68, 425–458.
Daniels, M. J., Chrispeels, M. J., and Yeager, M. (1999) Projection structure of a plant vacuole membrane aquaporin by electron cryo-crystallography. J. Mol. Biol. 294, 1337–1349.
Niemietz, C. M. and Tyerman, S. D. (1997) Characterization of water channels in wheat root membrane vesicles. Plant Physiol. 115, 561–567.
Charras, G. T., Yarrow, J. C., Horton, M. A., et al. (2005) Non-equilibration of hydrostatic pressure in blebbing cells. Nature 435, 365–369.
Mathur, J. (2006) Local interactions shape plant cells. Curr. Op. Cell Biol. 18, 40–46.
Lovy-Wheeler, A., Wilsen, K. L., Baskin, T. L. and Hepler, P. K. (2005). Enhanced fixation reveals the apical cortical fringe of actin filaments as a consistent feature of the pollen tube. Planta 221, 95–104.
Lancelle, S. A. and Hepler, P. K. (1992) Ultrastructure of freeze-substituted pollen tubes of Lilium longiflorum. Protoplasma 167, 215–230.
Duman, J. G., Lee, E., Lee, G. Y. et al. (2004) Membrane fusion correlates with surface charge in exocytic vesicles. Biochemistry 43, 7924–7939.
Morris, C. E., Wang, J. A., and Markin, B. S. (2003) The invagination of excess surface area by shrinking neurons. Biophys. J. 85, 223–235.
Kung, C. (2005) A possible unifying principle for mechanosensation. Nature 436, 647–654.
Martinac, B. (2004) Mechanosensitive ion channels: molecules of mechanotransduction. J. Cell Sci. 117, 2449–2460.
Mizuno, S. (2005) A novel method for assessing effects of hydrostatic fluid pressure on intracellular calcium: a study with bovine articular chondrocytes. Am. J. Physiol. Cell Physiol. 288, C329-C337.
Yeung, C. H., Barfield, J. P., and Cooper, T. G. (2005) The role of anion channels and Ca2+ in addition to K+ channels in the physiological volume regulation of murine spermatozoa. Mol. Reprod. Dev. 71, 368–379.
Arniges, M., Vazquez, E., Fernandez-Fernandez, J. M., and Valverde, M. A. (2004) Swelling-activated Ca2+ entry via TRPV4 channel is defective in cystic fibrosis airway epithelia. J. Biol. Chem. 279, 54062–54068.
Okada, Y., Maeno, E., Shimizu, T., et al., (2001) Receptormediated control of regulatory volume decrease (RVD) and apoptotic volume decrease (AVD). J. Physiol. Lond 532, 3–16.
Pasantes-Morales, H., Cardin, V., and Tuz, K. (2000) Signaling events during swelling and regulatory volume decrease. Neurochem. Res. 25, 1301–1314.
Chao, P. G., Tang, Z., Angelini, E., et al. (2005) Dynamic osmotic loading of chondrocytes using a novel microfluidic device. J. Biomechanics 38, 1273–1281.
Heidecker, M., Wener, L. H., Binder, K.-A. and Zimmerman, U. (2003) Turgor pressure changes trigger characteristic changes in the electrical conductance of the tonoplast and the plasmalemma of the marine alga Valonia utricularis. Plant Cell Environ. 26, 1035–1051.
Shabala, S., Babourina, O., and Newman, I. (2000) Ion-specific mechanisms of osmoregulation in bean mesophyll cells. J. Exp. Bot. 51, 1243–1253.
Okada, Y. (2004) Ion channels and transporters involved in cell volume regulation and sensor mechanisms. Cell Biochem. Biophys. 41, 233–258.
Wehner, F., Olsen, H., Tinel, H., et al. (2003) Cell volume regulation: osmolytes, osmolyte transport, and signal transduction. Rev. Physiol. Biochem. Pharmacol. 148, 1–80.
Dutta, R. and Robinson, K. R. (2004) Identification and characterization of stretch-activated ion channels in pollen protoplasts. Plant Physiol. 135, 1398–1406.
Mendgen K., Hahn, M., and Deising, H. (1996) Morphogenesis and mechanisms of penetration by plant pathogenic fungi. Annu. Rev. Phytopathol. 34, 367–386.
Money, N. P. and Howard, R. J. (1996) Confirmation of a link between fungal pigmentation, turgor pressure, and pathogenicity using a new method of turgor measurement. Fungal Genet. Biol. 20, 217–227.
Talbot, N. J. (1995) Having a blast: exploring the pathogenicity of Magnaporthe grisea. Trends Microbiol. 3, 9–16.
Money, N. P. Osmotic adjustment and the role of turgor in mycelial fungi. In: The Mycota, Vol. 1: Growth, Differentiation and Sexuality (Wessels, J. G. H. and Meinhardt, F., eds). Springer-Verlag, New York, 1994, pp. 67–81.
Money, N. P., Davis, C. M., and Ravishankar, J. P. (2004) Biomechanical evidence for convergent evolution of the invasive growth processes among fungi and oomycete water molds. Fungal Genet. Biol. 41, 872–876.
Franks, P. J. (2004) Stomatal control and hydraulic conductance, with special reference to tall trees. Tree Physiol. 24, 865–878.
Schroeder, J. I., Allen, G. J., Hugouvieux, V., et al. (2001) Guard cell signal transduction. Annu. Rev. Plant Physiol. Plant Mol. Biol. 52, 627–658.
Liu, K. and Luan, S. (1998) Voltage-dependent K+ channels as targets of osmosensing in guard cells. Plant Cell 10, 1957–1970.
Assmann, S. M. (1993) Signal transduction in guard cells. Annu. Rev. Cell Biol. 9, 345–375.
Schroeder, J. I. and Hedrich, R. (1989) Involvement of ion channels and active transport in osmoregulation and signaling of higher plant cells. Trends Biochem. Sci. 14, 187–192.
Suh, S., Moran, N., and Lee, Y. (2000) Blue light activates potassium efflux channels in flexor cells from Samanea saman motor organs via two mechanisms. Plant Physiol. 123, 833–843.
Kim, H. Y., Cote, G. G., and Crain, R. C. (1996) Inositol 1,4,5-trisphosphate may mediate closure of K+ channels by light and darkness in Samanea saman motor cells. Planta 198, 279–287.
Antkowiak, B., Mayer, W. E., and Engelmann, W. (1991) Oscillations of the membrane-potential of pulvinar motor cells in situ in relation to leaflet movements of Desmodium motorium. J. Exp. Bot. 42, 901–910.
Satter, R. L., Morse, M. J., Lee, Y., et al. (1998) Light-and clock-controlled leaflet movements in Samanea saman: a physiological, biophysical and biochemical analysis. Bot. Acta 101, 205–213.
Siefritz, F., Otto, B., Bienert, G. P., et al. (2004) The plasma membrane aquaporin NtAQP1 is a key component of the leaf unfolding mechanism in tobacco. Plant J. 37, 147–155
Tyerman, S. D., Niemietz, C. M. and Bramley, H. (2002) Plant aquaporins: multifiunctional water and solute channels with expanding roles. Plant Cell Environ. 25, 173–194.
Siefritz, F., Biela, A., Eckert, M., et al. (2001) The tobacco plasma membrane aquaporin NtAQP1. J. Exp. Bot. 52, 1953–1957.
Ruiter, R. K., Vaneldik, G. J., Vanherpen, M. M. A., et al. (1997) Expression in anthers of two genes encoding Brassica oleracea transmembrane channel proteins. Plant Mol. Biol. 34, 163–168.
Lush, W. M., Grieser, F., and Wolters-Arts, M. (1998) Directional guidance of Nicotiana alata pollen tubes in vitro and on the stigma. Plant Physiol. 118, 733–741.
Wolters-Arts, M., Lush, W. M., and Mariani, C. (1998) Lipids are required for directional pollen-tube growth. Nature 392, 818–821.
Alves, A. A. C. and Setter, T. L. (2004) Response of cassava leaf area expansion to water deficit: cell proliferation, cell expansion and delayed development. Ann. Bot. 94, 605–613.
Fricke, W. (2002) Biophysical limitation of cell elongation in cereal leaves. Ann. Bot. 90, 157–167.
Siefritz, F., Tyree, M. T., Lovisolo C., et al. (2002) PIP1 plasma membrane aquaporins in tobacco: from cellular effects of function in plants. Plant Cell 14, 869–876.
Ikeda, T., Nonami, H., Fukuyama, T., and Hashimoto, Y. (1999) Hydraulic contribution in cell elongation of tissue-cultured plants: growth retardation induced by osmotic and temperature stresses and addition of 2,4-dichlorophenoxyacetic acid and benzylaminopurine. Plant Cell Environ. 22, 899–912.
Matyssek, R., Maruyama, S., and Boyer, J. S. (1991) Growth-induced water potentials may mobilize internal water for growth. Plant Cell Environ. 14, 917–923.
Frixione, E., Ruiz, L., Cerbon, J., and Undeen, A. H. (1997) Germination of Nosema algerae (Microspora) spores: conditional inhibition by D2O, ethanol and Hg2+ suggests dependence of water influx upon membrane hydration and specific transmembrane pathways. J. Eukaryot. Microbiol. 44, 109–116.
Undeen, A. H. and Frixione, E. (1990) The role of osmotic pressure in the germination of Nosema algerae spores. J. Protozool. 37, 561–567.
Lew, R. R., Levina, N. N., Walker, S. K., and Garrill, A. (2004) Turgor regulation in hyphal organisms. Fungal Genet. Biol. 41, 1007–1015.
Money, N. P. (1997) Wishful thinking of turgor revisited: the mechanics of fungal growth. Fungal Genet. Biol. 21, 173–187.
Harold, F. M., Harold, R. L., and Money, N. P. (1995) What forces drive cell-wall expansion. Can J. Bot. 73, S379-S383.
Harold, R. L., Money, N. P., and Harold, F. M. (1996) Growth and morphogenesis in Saprolegnia ferax: is turgor required? Protoplasma 191, 105–114.
Money, N. P. (1995) Turgor pressure and the mechanics of fungal penetration. Can. J. Bot. 73, S96-S102.
Lew, R. R. (2005) Mass flow and pressure-driven hyphal extension in Neurospora crassa. Microbiol. 151, 2685–2692.
Nieuwland, J., Feron, R., Huisman, B. A. H., et al. (2005) Lipid transfer proteins enhance cell wall extension in tobacco. Plant Cell, 17, 2009–2019.
Cosgrove, D. J., Bedinger, P., and Durachko, D. M. (1997) Group I allergens of grass pollen as cell wall-loosening agents. Proc. Natl. Acad. Sci. U. S. A. 94, 6559–6564.
Lord, E. M. (2003) Adhesion and guidance in compatible polination. J. Exp. Bot. 54, 47–54.
Shabala, S., Shabala, L., Gradmann, D., et al. (2006) Oscillations in plant membrane transport: model predictions experimental validation, and physiological implications. J. Exp. Bot. 57, 171–184
Gilden, D. L. (2001) Cognitive emissions of 1/f noise. Psychol. Rev. 108, 33–56.
Agu, M. and Yamada, M. (1998) Short-time information entropy as a complexity measure. Jap. J. Applied. Phys. Part 2-Lett. 37, L1415-L1417.
Gilden, D. L., Thronton, T., and Mallon, M. W. (1995) 1/f noise in human cognition. Science 267, 1837–1839.
Schrader, B., Klump, H. H., Schenzel, K., and Schulz, H. (1999) Non-destructive NIR FT Raman analysis of plants. J. Mol. Struct. 509, 201–212.
Schrader, B. Infrared and Raman Spectroscopy. VCH Publishers, Weinheim, 1995.
Author information
Authors and Affiliations
Corresponding author
Rights and permissions
About this article
Cite this article
Zonia, L., Müller, M. & Munnik, T. Hydrodynamics and cell volume oscillations in the pollen tube apical region are integral components of the biomechanics of Nicotiana tabacum pollen tube growth. Cell Biochem Biophys 46, 209–232 (2006). https://doi.org/10.1385/CBB:46:3:209
Issue Date:
DOI: https://doi.org/10.1385/CBB:46:3:209