Abstract
The ability of sperm to self-propel through the female reproductive tract is essential for natural fertilisation. Despite this fact, manual assessments of motility are limited in scope and computer-aided sperm analysis (CASA) systems are not routinely used in clinical practice. One significant factor hindering the clinical use of CASA systems is the lack of evidence linking motility measures and fertility outcomes. To progress these technologies, we need to address the variations in the way samples are prepared and imaged, and whether current kinematic parameters provide the physiological insight necessary for establishing these links. In this manuscript, we discuss how preparation (sample viscosity, temperature, concentration), acquisition (chamber depth, frame rate, duration) and analysis can dramatically affect CASA results. With the aim of advancing the clinical application of CASA, we outline the requirements for obtaining measurements that can be compared between samples and systems. We further highlight how the introduction of flagellar tracking can form the basis of increasingly insightful diagnostics; by combining kinematic data with mathematical modelling experimentally intractable details can be uncovered, such as metabolic requirements of motility from a single cell to the population level.
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Achikanu C, Correia J, Guidobaldi H, Giojalas L, Barratt C, Da Silva S, Publicover S (2019) Continuous behavioural ‘switching’ in human spermatozoa and its regulation by Ca2+-mobilising stimuli. Mol Hum Reprod 25(8):423–432
Afzelius B (1959) Electron microscopy of the sperm tail results obtained with a new fixative. J Cell Biol 5(2):269–278
Bompart D, Garćıa-Molina A, Valverde A, Caldeira C, Yániz J, de Murga M, Soler C (2018) CASA-mot technology: how results are affected by the frame rate and counting chamber. Reprod Fertil Dev 30(6):810–819
Boryshpolets S, Pérez-Cerezales S, Eisenbach M (2015) Behavioral mechanism of human sperm in thermotaxis: a role for hyperactivation. Hum Reprod 30(4):884–892
Brechet L, Lucas M-F, Doncarli C, Farina D (2007) Compression of biomedical signals with mother wavelet optimization and best-basis wavelet packet selection. IEEE Trans Biomed Eng 54(12):2186–2192
Cancel A, Lobdell D, Mendola P, Perreault S (2000) Objective evaluation of hyperactivated motility in rat spermatozoa using computer-assisted sperm analysis. Hum Reprod 15(6):1322–1328
Curtis M, Kirkman-Brown J, Connolly T, Gaffney E (2012) Modelling a tethered mammalian sperm cell undergoing hyperactivation. J Theor Biol 309:1–10
Delmotte B, Climent E, Plouraboúe, F. (2015a) A general formulation of bead models applied to flexible fibers and active filaments at low Reynolds number. J Comput Phys 286:14–37
Delmotte B, Keaveny E, Plouraboué F, Climent E (2015b) Large-scale simulation of steady and time-dependent active suspensions with the force-coupling method. J Comput Phys 302:524–547
Dillon R, Fauci L, Omoto C (2003) Mathematical modeling of axoneme mechanics and fluid dynamics in ciliary and sperm motility. Dynam Cont Dis A 10:745–758
Duffy B, Thiyagalingam J, Walton S, Smith D, Trefethen A, Kirkman-Brown J, Gaffney E, Chen M (2013) Glyph-based video visualization for semen analysis. IEEE Trans Vis Comput Graph 21(8):980–993
Esfandiari N, Saleh R, Blaut A, Sharma R, Nelson D, Thomas A, Falcone T, Agarwal A (2002) Effects of temperature on sperm motion characteristics and reactive oxygen species. Int J Fertil Womens Med 47(5):227–235
Fawcett D, Porter K (1954) A study of the fine structure of ciliated epithelia. J Morphol 94(2):221–281
Gallagher M, Smith D (2018) Meshfree and efficient modeling of swimming cells. Phys Rev Fluids 3(5):053101
Gallagher M, Cupples G, Ooi E, Kirkman-Brown J, Smith D (2019) Rapid sperm capture: high-throughput flagellar waveform analysis. Hum Reprod 34:1173–1185
Gillies E, Cannon R, Green R, Pacey A (2009) Hydrodynamic propulsion of human sperm. J Fluid Mech 625:445–474
Goodson S, Zhang Z, Tsuruta J, Wang W, O’Brien D (2011) Classification of mouse sperm motility patterns using an automated multiclass support vector machines model. Biol Reprod 84(6):1207–1215
Gray J, Hancock G (1955) The propulsion of sea-urchin spermatozoa. J Exp Biol 32(4):802–814
Hall-McNair A, Gallagher M, Montenegro-Johnson T, Gadêlha H, Smith D (2019) Efficient implementation of elastohydrodynamics via integral operators. Phys Rev Fluids 4:113101
Hansen J, Rassmann S, Jikeli J, Wachten D (2019) Spermq – a simple analysis software to comprehensively study flagellar beating and sperm steering. Cell 8(1):10
Hiramoto Y, Baba S (1978) A quantitative analysis of flagellar movement in echinoderm spermatozoa. J Exp Biol 76(1):85–104
Holt W, Moore H, Hillier S (1985) Computer-assisted measurement of sperm swimming speed in human semen: correlation of results with in vitro fertilization assays. Fertil Steril 44(1):112–119
Hooker R (1901) Correlation of the marriage-rate with trade. J R Stat Soc 64(3):485–492
Ishimoto K, Gaffney E (2016) Mechanical tuning of mammalian sperm behaviour by hyperactivation, rheology and substrate adhesion: a numerical exploration. J R Soc Interface 13(124):20160633
Ishimoto K, Gadêlha H, Gaffney E, Smith D, Kirkman-Brown J (2018) Human sperm swimming in a high viscosity mucus analogue. J Theor Biol 446:1–10
Kaneko T, Mōri T, Ishijima S (2007) Digital image analysis of the flagellar beat of activated and hyperactivated suncus spermatozoa. Mol Reprod Dev 74(4):478–485
Katz D, Berger S (1980) Flagellar propulsion of human sperm in cervical mucus. Biorheology 17(1–2):169–175
Katz D, Overstreet J (1981) Sperm motility assessment by videomicrography. Fertil Steril 35(2):188–193
Lewis S (2007) Is sperm evaluation useful in predicting human fertility? Reproduction 134(1):31–40
Lin J, Nicastro D (2018) Asymmetric distribution and spatial switching of dynein activity generates ciliary motility. Science 360(6387):eaar1968
Machin K (1958) Wave propagation along flagella. J Exp Biol 35(4):796–806
Mallat S (1999) A wavelet tour of signal processing. Elsevier, Amsterdam
Maŕın-Briggiler C, Teźon J, Miranda P, Vazquez-Levin M (2002) Effect of incubating human sperm at room temperature on capacitation-related events. Fertil Steril 77(2):252–259
McPartlin L, Suarez S, Czaya C, Hinrichs K, Bedford-Guaus S (2009) Hyperactivation of stallion sperm is required for successful in vitro fertilization of equine oocytes. Biol Reprod 81(1):199–206
Mortimer S (2000) CASA—practical aspects. J Androl 21(4):515–524
Mortimer S, van der Horst G, Mortimer D (2015) The future of computer-aided sperm analysis. Asian J Androl 17(4):545
Neal C, Hall-McNair A, Gallagher M, Kirkman-Brown J, Smith D (2020) Doing more with less: the flagellar end piece enhances the propulsive effectiveness of spermatozoa. Phys Rev Fluids 5(7):073101
Nosrati R, Driouchi A, Yip C, Sinton D (2015) Two-dimensional slither swimming of sperm within a micrometre of a surface. Nat Commun 6:8703
Nyquist H (1928) Certain topics in telegraph transmission theory. Trans Am Inst Electr Eng 47(2):617–644
Ohmuro J, Ishijima S (2006) Hyperactivation is the mode conversion from constant-curvature beating to constant-frequency beating under a constant rate of microtubule sliding. Mol Reprod Dev 73(11):1412–1421
Ola B, Afnan M, Papaioannou S, Sharif K, Bj̈orndahl L, Coomarasamy A (2003) Accuracy of sperm–cervical mucus penetration tests in evaluating sperm motility in semen: a systematic quantitative review. Hum Reprod 18(5):1037–1046
Olson S, Suarez S, Fauci L (2011) Coupling biochemistry and hydrodynamics captures hyperactivated sperm motility in a simple flagellar model. J Theor Biol 283(1):203–216
Ooi E, Smith D, Gadêlha H, Gaffney E, Kirkman-Brown J (2014) The mechanics of hyperactivation in adhered human sperm. Roy Soc Open Sci 1(2):140230
Phan-Thien N, Tran-Cong T, Ramia M (1987) A boundary-element analysis of flagellar propulsion. J Fluid Mech 184:533–549
Rafiee J, Rafiee M, Prause N, Schoen M (2011) Wavelet basis functions in biomedical signal processing. Expert Syst Appl 38(5):6190–6201
Satir P (1968) Studies on cilia: III. Further studies on the cilium tip and a “sliding filament” model of ciliary motility. J Cell Biol 39(1):77–94
Schoeller S, Townsend A, Westwood T, Keaveny E (2021) Methods for suspensions of passive and active filaments. J Comp Phys 424:109846
Smith D, Gaffney E, Blake J, Kirkman-Brown J (2009a) Human sperm accumulation near surfaces: a simulation study. J Fluid Mech 621:289–320
Smith D, Gaffney E, Gadêlha H, Kapur N, Kirkman-Brown J (2009b) Bend propagation in the flagella of migrating human sperm, and its modulation by viscosity. Cell Motil Cytoskel 66(4):220–236
Stauss C, Votta T, Suarez S (1995) Sperm motility hyperactivation facilitates penetration of the hamster zona pellucida. Biol Reprod 53(6):1280–1285
Suarez S (2008) Control of hyperactivation in sperm. Hum Reprod Update 14(6):647–657
Talarczyk-Desole J, Berger A, Taszarek-Hauke G, Hauke J, Pawelczyk L, Jedrzejczak P (2017) Manual vs. computer-assisted sperm analysis: can CASA replace manual assessment of human semen in clinical practice? Ginekol Pol 88(2):56–60
Tomlinson M, Naeem A (2018) CASA in the medical laboratory: CASA in diagnostic andrology and assisted conception. Reprod Fertil Dev 30(6):850–859
Unser M, Aldroubi A (1996) A review of wavelets in biomedical applications. Proc IEEE 84(4):626–638
van der Horst G, du Plessis S (2017) Not just the marriage of Figaro: but the marriage of WHO/ESHRE semen analysis criteria with sperm functionality. Adv Androl 4:6–21
van der Horst G, Maree L, du Plessis S (2018) Current perspectives of CASA applications in diverse mammalian spermatozoa. Reprod Fertil Dev 30(6):875–888
Walker B, Ishimoto K, Wheeler R (2019) Automated identification of flagella from videomicroscopy via the medial axis transform. Sci Rep 9(1):5015
Wolf D, Hagopian S, Ishijima S (1986) Changes in sperm plasma membrane lipid diffusibility after hyperactivation during in vitro capacitation in the mouse. J Cell Biol 102(4):1372–1377
World Health Organisation (2010) WHO laboratory manual for the examination of human semen and sperm-cervical mucus interaction, 5th edn. Cambridge University Press, Cambridge
Yanagimachi R (1970) The movement of golden hamster spermatozoa before and after capacitation. Reproduction 23(1):193–196
Acknowledgements
The ongoing support of patients and staff at the Birmingham Women’s and Children’s NHS Foundation Trust are fundamental to our research work. The authors gratefully acknowledge funding from the Engineering and Physical Sciences Research Council, Healthcare Technologies Challenge Award (EP/N021096/1). Jackson Kirkman-Brown is funded by a National Institute of Health Research (NIHR), and Health Education England, Senior Clinical Lectureship Grant: The role of the human sperm in healthy live birth (NIHRDH-HCS SCL-2014-05-001). This article presents independent research funded in part by the National Institute for Health Research NIHR and Health Education England. The views expressed are those of the authors and not necessarily those of the NHS, the NIHR or the Department of Health.
Ethical approval: All donors were recruited in accordance with the Human and Embryology Authority Code of Practice (version 7) and gave informed consent (South Birmingham LREC 2003/239 and East Midlands REC 13/EM/0272).
Conflict of interest: The authors declare no competing interests.
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Appendix
Appendix
The characteristic sperm tracks presented in this paper are taken from semen samples provided by unscreened normozoospermic donors recruited at Birmingham Women’s and Children’s NHS Foundation Trust after giving informed consent. Full details of the experimental procedures for each cell shown in Figs. 1–7 can be found in this appendix.
Figure 1—Cells were suspended in supplemented Earle’s balanced salt solution (sEBSS) without phenol red, and supplemented with 2.5 mM Na pyruvate and 19 mM Na lactate (06-2010-03-1B; Biological Industries, Kibbutz Beit HaEmek, Israel), and 0.3% weight/volume charcoal delipidated bovine serum albumin. Cells were imaged in a 10 μm depth chamber (10-01-04-B-CE; Leja Products B.V., Nieuw-Vennep, The Netherlands) using an Olympus (BX-50) microscope and negative-phase contrast microscopy (objective 20× 0.40 Ph1 BM ∞/0.17 WD 1.2), and recorded using a Hamamatsu Photonics C9300 CCD camera (pixel size 7.4 μm at 285.2 Hz).
Figure 2—(a) Cells were selected using a swim-up, where a 500 μL aliquot of supplemented Earle’s balanced salt solution (sEBSS) without phenol red, and supplemented with 2.5 mM Na pyruvate and 19 mM Na lactate (06-2010-03-1B; Biological Industries, Kibbutz Beit HaEmek, Israel), and 0.3% weight/volume charcoal delipidated bovine serum albumin was placed in a 5 mL round-bottom tube (Corning, Falcon 352058). A 300 μL aliquot of semen was pipetted to the bottom of the tube, inclined and left in the incubator for 30 min at 37 °C. Cells were imaged in a 10 μm depth chamber using a Nikon (Eclipse 80i) microscope and negative-phase contrast microscopy at 10× magnification (10× 0.2 Ph1 BM ∞/-WD7.0) and an Andor Zyla 5.5 (Andor, Oxford UK) microscopy camera at 200 Hz with pixel size 6.5 μm × 6.5 μm.
Figure 2—(b) Cells were suspended in supplemented Earle’s balanced salt solution (sEBSS) without phenol red and supplemented with 2.5 mM Na pyruvate and 19 mM Na lactate (06-2010-03-1B; Biological Industries, Kibbutz Beit HaEmek, Israel), and 0.3% weight/volume charcoal delipidated bovine serum albumin, with the addition of 1% methylcellulose (M0512, Sigma-Aldrich, Poole, UK, specified so that an aqueous 2% solution gives a nominal viscosity of 4000 centipoise or 4 Pa s at 20 °C). The cells were loaded by capillary action into flat-sided borosilicate capillary tubes (VITROTUBES, 2540, Composite Metal Services, Ilkley, UK) with length 50 mm and inner dimensions 4 × 0.4 mm. One end of the tube was sealed with CRISTASEAL (Hawksley, Sussex, UK #01503-00). Cells were selected for imaging by immersing the open end of the capillary tube into a 1.5 mL Beem capsule (Agar Scientific, UK) containing a 200 μL aliquot of raw semen, within 30 min of sample production. Incubation was performed for 30 min at 37 °C in 6% CO2. Cells were imaged at 2 cm migration distance into the capillary tube and in the surface accumulated layer 10–20 μm from the inner surface of the capillary tube at 10× magnification using a Nikon (Eclipse 80i) microscope and negative-phase contrast microscopy and an Andor Zyla microscopy camera (pixel size 6.5 × 6.5 μm) at 200 Hz.
Figure 3—The sample was counted according to WHO guidelines (WHO 2010) and diluted to a concentration of 10 M/mL in of supplemented Earle’s balanced salt solution (sEBSS) without phenol red, and supplemented with 2.5 mM Na pyruvate and 19 mM Na lactate (06-2010-03-1B; Biological Industries, Kibbutz Beit HaEmek, Israel), and 0.3% weight/volume charcoal delipidated bovine serum albumin. Cells were imaged in a 10 μm depth chamber using a Nikon (Eclipse 80i) microscope and negative-phase contrast microscopy (objectives 10× 0.2 Ph1 BM ∞/-WD7.0), using a Basler Microscopy ace camera (acA 1300-200uc) at 169 Hz with pixel size 4.8 × 4.8 μm, using Pylon Viewer (v.5.0.11.10913, Basler AG, Ahrensburg, Germany).
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Cupples, G., Gallagher, M.T., Smith, D.J., Kirkman-Brown, J.C. (2021). Heads and Tails: Requirements for Informative and Robust Computational Measures of Sperm Motility. In: Björndahl, L., Flanagan, J., Holmberg, R., Kvist, U. (eds) XIIIth International Symposium on Spermatology. Springer, Cham. https://doi.org/10.1007/978-3-030-66292-9_21
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