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  • Methodology
  • Open Access

The effect of ultrasound-related stimuli on cell viability in microfluidic channels

  • 1Email author,
  • 1, 2,
  • 1,
  • 1,
  • 3,
  • 2 and
  • 1
Contributed equally
Journal of Nanobiotechnology201311:20

Received: 17 June 2013

Accepted: 17 June 2013

Published: 28 June 2013



In ultrasonic micro-devices, contrast agent micro-bubbles are known to initiate cavitation and streaming local to cells, potentially compromising cell viability. Here we investigate the effects of US alone by omitting contrast agent and monitoring cell viability under moderate-to-extreme ultrasound-related stimuli.


Suspended H9c2 cardiac myoblasts were exposed to ultrasonic fields within a glass micro-capillary and their viability monitored under different US-related stimuli. An optimal injection flow rate of 2.6 mL/h was identified in which, high viability was maintained (~95%) and no mechanical stress towards cells was evident. This flow rate also allowed sufficient exposure of cells to US in order to induce bioeffects (~5 sec), whilst providing economical sample collection and processing times. Although the transducer temperature increased from ambient 23°C to 54°C at the maximum experimental voltage (29 V pp ), computational fluid dynamic simulations and controls (absence of US) revealed that the cell medium temperature did not exceed 34°C in the pressure nodal plane. Cells exposed to US amplitudes ranging from 0–29 V pp , at a fixed frequency sweep period (tsw = 0.05 sec), revealed that viability was minimally affected up to ~15 V pp . There was a ~17% reduction in viability at 21 V pp , corresponding to the onset of Rayleigh-like streaming and a ~60% reduction at 29 V pp , corresponding to increased streaming velocity or the potential onset of cavitation. At a fixed amplitude (29 V pp ) but with varying frequency sweep period (tsw = 0.02-0.50 sec), cell viability remained relatively constant at tsw ≥ 0.08 sec, whilst viability reduced at tsw < 0.08 sec and minimum viability recorded at tsw = 0.05 sec.


The absence of CA has enabled us to investigate the effect of US alone on cell viability. Moderate-to-extreme US-related stimuli of cells have allowed us to discriminate between stimuli that maintain high viability and stimuli that significantly reduce cell viability. Results from this study may be of potential interest to researchers in the field of US-induced intracellular drug delivery and ultrasonic manipulation of biological cells.


  • Ultrasound (US)
  • Micro-device
  • Cardiac myoblasts
  • Cell viability


In ultrasonic cell stimulation micro-devices, the inclusion of ultrasound (US) contrast agent (CA) to enhance US bioeffects or increase cell membrane permeability is common [1]. However, CAs can initiate cavitation and streaming [2] local to cells, potentially compromising cell viability [3, 4]. Thus, higher cell viability is likely to be maintained in the absence of CA [57]. In our previous study we reported on ultrasonically induced membrane poration of a cardiac myoblast cell line (H9c2) in the absence of CA by generating an ultrasonic field within a biocompatible glass micro-capillary [3]. Notably, high cell viability was maintained in the absence of CA [3]. Following a similar approach, Longsine-Parker et al. recently demonstrated effective cell membrane poration in a microfluidic device by combining the action of electric fields and US waves in a CA-free environment [8].

Here we investigate US-“alone”-related physical stimuli of H9c2 cells. We expose suspended cells to gentle, moderate and extreme US amplitudes. Extreme amplitudes also initiate an increase in transducer temperature; therefore we also investigated the effect of US-related temperature increase on cell viability. Cell viability was also measured following infusion into the micro-device at varying flow regimes in order to optimise the flow rate. Of particular interest to us is the effect of frequency sweeping on cells as a means of controllably stressing cells and potentially increasing membrane permeability.


Cells were subjected to a variety of US-related stimuli (summarised in Table 1) in order to assess the effect of US alone on cell viability in the absence of CA.
Table 1

Summary of the experiments performed to investigate the effect of US-related stimuli on H9c2 cell viability


Operating conditions


Flow rate through the micro-capillary

Inlet flow rate: 1.3–13.0 mL/h

Figure 3

US-induced thermal variations

PZT temperature measurements and CFD simulations of fluid temperature distribution

Figure 4a

Controls (correspondent PZT temperatures, absence of US)

Figure 4b

Amplitude variations

Driving voltage: 6–29 V pp

Figure 5

Sweep period variations

Sweep period: 0.02–0.50 sec

Figure 1

At 2.6 mL/h viability was uncompromised, likely due to low mechanical stress (Figure 1). This flow rate also provided economical sample collection and processing times whilst allowing sufficient exposure of cells to US (texp  5 sec) for generating observable bioffects. Furthermore, no cell trapping was evident, providing homogeneous exposure of cells to US.
Figure 1
Figure 1

Effect of fluid flow rate on cell viability. Cell viability was measured at flow rates ranging from 1.3-13.0 mL/h. At 2.6 mL/h cell viability was uncompromised (control viability = 97±1%), cells were allowed sufficient US exposure (texp 5 sec), and trapping was not evident (n = 3).

During US applied at the maximum experimental voltage, 29 V pp , the transducer temperature was noted to increase from ambient 23°C to a biologically unfavourable 54°C. However, CFD simulations revealed that the temperature of the liquid medium at the capillary centerline only increased up to a maximum of ~34°C (Figure 2a). To validate the simulations, control experiments (absence of US), replacing the transducer with a hot plate fixed at 54°C, revealed that cell viability was minimally affected (92.12±2.94%), while during US exposure at 29 Vpp, viability reduced to 43.28±5.54% (Figure 2b). This suggests that PZT heating per se did not compromise cell viability. However, the CFD simulations did not take into account the effect of acoustic streaming on heat transfer within the fluidic domain, which may have contributed to the reduction in cell viability.
Figure 2
Figure 2

Effect of temperature on cell viability. a] Fluid temperature profile along the glass microchannel centerline and contours of fluid temperature determined computationally. b] Cell viability during US exposure (black squares), and absence of US (red circle) with PZT substituted by a hot plate at corresponding temperatures (n = 4).

Cell viability was measured immediately following exposure to US amplitudes ranging from 0–29 V pp , using a fixed frequency sweep period of 0.05 sec. Figure 3 demonstrates that cell viability was not compromised up to ~15 V pp . However a ~17% reduction in cell viability was measured at 21 V pp , corresponding to the onset of streaming, assigned as Rayleigh-like (observed with fluorescent tracers under static conditions), characterised by the formation of toroidal axially centred vortices [10]. A ~60% viability reduction was measured at 29 V pp , corresponding to an observed increase of the streaming velocity. Furthermore, the acoustic pressure (measured by drop-voltage analysis at a fixed f = 2.18 MHz) was ~2.05×104×V pp Pa. This corresponded to pressures in the range 0.12–0.59 MPa, thus suggesting that cavitation may have occurred at V pp > 20. Notably, Apfel and Holland determined a minimum pressure threshold of ~0.4 MPa for cavitation to occur in water, at a frequency of ~2 MHz [6, 11].
Figure 3
Figure 3

Effect of US amplitude on cell viability. Up to ~15 V pp cell viability was unaffected, a ~17% reduction in viability was measured at 21 V pp (corresponding to the onset of Rayleigh-like streaming) and a ~60% reduction was measured at 29 V pp (corresponding to increased streaming velocities) (n = 4).

At a fixed amplitude (29 V pp ) but varying the sweep period (tsw = 0.02-0.50 sec), cell viability was virtually unaffected by frequency sweep periods tsw ≥ 0.08 sec. However, at sweep periods tsw < 0.08 sec cell viability decreased, with minimum viability (~41%) measured at tsw = 0.05 sec (Figure 4a). Under identical acoustic conditions, 20 μ m diameter fluorescent beads were observed to rapidly oscillate across a relatively smaller distance away from the nodal plane at tsw = 0.1 sec, compared with tsw = 0.5 sec where bead oscillation was visibly slower over increased distances away from the nodal plane (Figure 4b).
Figure 4
Figure 4

Effect of frequency sweep on cell viability and bead oscillatory dynamics. a] Cell viability was unaffected by tsw ≥ 0.08 sec but decrease ≥ 0.08 sec using a frequency range: 2.13-2.40 MHz and at a fixed 29 V pp . b] Oscillatory dynamics of 20 μ m diameter fluorescent polystyrene beads at a sweep period of 0.5 and 0.1 sec.


The effect of individual US-related physical parameters (fluid flow rate, US heat generation, amplitude and frequency sweep period) on H9c2 cell viability was assessed within a microfluidic device. The optimised flow rate did not inflict any detectable mechanical stress, and thus high cell viability was maintained. Moreover cells were allowed sufficient exposure to US in order to elicit bioeffects, whilst providing economical sample processing times and minimising cell trapping. High cell viability was maintained at amplitudes where streaming was not evident. However, when more extreme amplitudes were employed, streaming velocities increased and cell viability significantly decreased. Extreme amplitudes also initiated an increase in PZT temperature, however cell viability was unaffected by this increase due to heat dissipation, confirmed by controls and CFD simulations. Longer duration frequency sweeps were identified to have little or no effect on cell viability, whereas short sweeps resulted in reduced cell viability. This effect may be attributed to mechanical stress generated by rapid oscillatory movements of the cell within the fluidic domain [12]. Notably, experiments with fluorescent tracer beads revealed that bead oscillation frequency increased with reducing the sweep interval, which may explain the reduction in cell viability at the shorter tsw. However, an in depth investigation into the effects of frequency sweeping on cell viability is currently underway in our laboratories.


Our CA-free investigation into the effects of US on cell viability has enabled us to discriminate between US-related stimuli that do not compromise cell viability and stimuli that significantly reduce cell viability within our micro-device. Our findings may be of potential interest to researchers in the field of US-induced intracellular drug delivery and ultrasonic manipulation of biological cells.


The micro-device (Figure 5a), comprising of a squared cross-section borosilicate glass micro-capillary (length: 50 mm, internal width: 300 μ m, wall thickness: 150 μ m; VitroCom, Ilkley, UK), was acoustically coupled to a piezoelectric transducer (PZT; PZ26 Ferroperm, Kvistgard, Denmark) using glycerol. The transducer (length: 40 mm, width: 9 mm and thickness: 1 mm) was fixed to a glass platform and driven by an RF power amplifier (240 L ENI, New York, USA) fed from a signal generator (TG103 TTI, Cambridgeshire, UK). A time varying ultrasonic field was generated within the capillary and the operating frequency determined through electrical impedance measurements (C-60 impedance analyser, Cypher Instruments Ltd., London, UK) of the capillary both air-filled and fluid-filled (Figure 2b).
Figure 5
Figure 5

Microfluidic device. a] device comprising of a squared cross-section glass capillary (length: 50 mm, internal width: 300 μ m and wall thickness: 150 μ m), coupled to a PZT transducer (length: 40 mm, width: 9 mm and thickness: 1 mm) and mounted on a glass platform. b] Modulus of impedance (Ω) for the air-filled and the liquid-filled micro-capillary, respectively. Frequency range: 2.13-2.40 MHz.

H9c2 cardiac myoblasts were grown in Dulbecco’s Modified Eagle Medium (DMEM) culture medium supplemented with 10% (v/v) foetal calf serum and 1% (v/v) penicillin-streptomycin (media and supplements purchased from Fisher Scientific, Loughborough, UK). Cells were maintained at 37°C, 5% CO2 in air with 95% humidity. Cells were routinely harvested and suspended at a density of 2×106 cells/mL in serum free DMEM within a 1 mL sterile, plastic syringe (BD Bioscience, Oxford, UK). Cells were infused into the device using a syringe pump (KD100, KD Scientific Inc., Holliston, USA) and subjected to ultrasound-related physical stimuli. Cells were captured in 1 mL sterile tubes, followed by counting and viability assessment using a Neubauer haemocytometer (depth: 0.1 mm, area: 0.04 mm2) and trypan blue exclusion dye. All viability measurements were in triplicate or greater.

To optimise the flow rate, cell viability was measured following infusion into the device at a range of flow rates (1.3-13.0 mL/h), which were prior calculated in order to: i) provide sufficient exposure of cells to US, ii) provide economical cell collection and processing times, iii) minimise flow-induced mechanical stress on cells and iv) minimise cell trapping.

To assess US-related thermal effects on cell viability, cells were infused into the device at a fixed flow rate (2.6 mL/h) and exposed to US (6–29 V pp ), whilst thermocouples were attached to the transducer, and temperatures recorded using a thermometer (HH11 Omega®, Manchester, UK). Controls were produced in the absence of US by replacing the transducer with a hot plate (Fisher Scientific, Loughborough, UK) at identical temperatures to the recorded transducer temperatures. Additionally, computational fluid dynamic (CFD) simulations were performed to predict the transfer of heat from the transducer to the cell medium within the capillary.

The effect of US amplitude on cell viability was investigated by varying the V pp , ranging from 0–29 V pp , using a fixed frequency sweep period of 0.05 sec in the frequency range 2.13-2.40 MHz. Additionally, flow visualisation experiments, using 1 μ m diameter fluorescent tracers (Polysciences, Inc., Warrington, USA), were performed to characterise the fluid dynamic environment under “gentle” (6 V pp ) to “extreme” (29 V pp ) US amplitudes. The acoustic pressure within the capillary was measured through drop-voltage analysis [9], using 20 μ m diameter fluorescent polystyrene beads. A fixed resonance frequency of 2.18 MHz was set in this case, due to the difficulty in obtaining acoustic pressure values during frequency sweeping.

The effect of frequency sweep duration on cell viability was investigated by varying the sweep period (0.02-0.50 sec) at a fixed voltage (29 V pp ).




We are very grateful to Agilent Technologies, Santa Clara, CA, USA for funding this research (University Relations Grant 2012, Gift# 2700).

Authors’ Affiliations

Electromechanical Engineering Group, Faculty of Engineering and the Environment, University of Southampton, Southampton, UK
Bioengineering Sciences Group, Faculty of Engineering and the Environment, University of Southampton, Southampton, UK
Faculty Institute for Cancer Sciences, Faculty of Medical and Health Sciences, Manchester Academic Health Science Centre, University of Manchester, Manchester, UK


  1. Le Gac S, Zwaan E, Van Den Berg A, Ohl C-D: Sonoporation of suspension cells with a single cavitation bubble in a microfluidic confinement. Lab Chip. 2007, 7 (12): 1666-1672. 10.1039/b712897p.View ArticleGoogle Scholar
  2. Collis J, Manasseh R, Liovic P, Tho P, Ooi A, Petkovic-Duran K, Zhu Y: Cavitation microstreaming and stress fields created by microbubbles. Ultrasonics. 2010, 50 (2): 273-279. 10.1016/j.ultras.2009.10.002.View ArticleGoogle Scholar
  3. Carugo D, Ankrett DN, Glynne-Jones P, Capretto L, Boltryk RJ, Zhang X, Townsend PA, Hill M: Contrast agent-free sonoporation: the use of an ultrasonic standing wave microfluidic system for the delivery of pharmaceutical agents. Biomicrofluidics. 2011, 5 (4): 044108-10.1063/1.3660352.View ArticleGoogle Scholar
  4. Brayman AA, Azadniv M, Cox C, Miller MW: Hemolysis of albunex-supplemented, 40% hematocrit human erythrocytes in vitro by 1-MHz pulsed ultrasound: Acoustic pressure and pulse length dependence. Ultrasound Med Biol. 1996, 22 (7): 927-938. 10.1016/0301-5629(96)00108-1.View ArticleGoogle Scholar
  5. Hultström J, Manneberg O, Dopf K, Hertz HM, Brismar H, Wiklund M: Proliferation and viability of adherent cells manipulated by standing-wave ultrasound in a microfluidic chip. Ultrasound Med Biol. 2007, 33 (1): 145-151. 10.1016/j.ultrasmedbio.2006.07.024.View ArticleGoogle Scholar
  6. Wiklund M: Acoustofluidics 12: Biocompatibility and cell viability in microfluidic acoustic resonators. Lab Chip. 2012, 12: 2018-2028. 10.1039/c2lc40201g.View ArticleGoogle Scholar
  7. Evander M, Johansson L, Lilliehorn T, Piskur J, Lindvall M, Johansson S, Almqvist M, Laurell T, Nilsson J: Noninvasive acoustic cell trapping in a microfluidic perfusion system for online bioassays. Anal Chem. 2007, 79 (7): 2984-2991. 10.1021/ac061576v.View ArticleGoogle Scholar
  8. Longsine-Parker W, Wang H, Koo C, Kim J, Kim B, Jayaraman A, Han A: Microfluidic electro-sonoporation: a multi-modal cell poration methodology through simultaneous application of electric field and ultrasonic wave. Lab Chip. 2013, 13: 2144-2152. 10.1039/c3lc40877a.View ArticleGoogle Scholar
  9. Glynne-Jones P, Boltryk RJ, Hill M, Zhang F, Dong L, Wilkinson JS, Melvin T, Harris NR, Brown T: Flexible acoustic particle manipulation device with integrated optical waveguide for enhanced microbead assays. Anal Sci. 2009, 25 (2): 285-291. 10.2116/analsci.25.285.View ArticleGoogle Scholar
  10. Sorando AC, Hawkes JJ, Fielden PR, González I: Patterns of particles aggregation and streaming in resonating fluids. AIP Conference Proceedings. 2012, 1433: 757.View ArticleGoogle Scholar
  11. Apfel RE, Holland CK: Gauging the likelihood of cavitation from short-pulse, low-duty cycle diagnostic ultrasound. Ultrasound Med Biol. 1991, 17 (2): 179-185. 10.1016/0301-5629(91)90125-G.View ArticleGoogle Scholar
  12. Radel S, McLoughlin A, Gherardini L, Doblhoff-Dier O, Benes E: Viability of yeast cells in well controlled propagating and standing ultrasonic plane waves. Ultrasonics. 2000, 38 (1): 633-637.View ArticleGoogle Scholar


© Ankrett et al.; licensee BioMed Central Ltd. 2013

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