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Willaert, R. Nanomotion Detection-Based AST. Encyclopedia. Available online: https://encyclopedia.pub/entry/8350 (accessed on 12 February 2026).
Willaert R. Nanomotion Detection-Based AST. Encyclopedia. Available at: https://encyclopedia.pub/entry/8350. Accessed February 12, 2026.
Willaert, Ronnie. "Nanomotion Detection-Based AST" Encyclopedia, https://encyclopedia.pub/entry/8350 (accessed February 12, 2026).
Willaert, R. (2021, March 30). Nanomotion Detection-Based AST. In Encyclopedia. https://encyclopedia.pub/entry/8350
Willaert, Ronnie. "Nanomotion Detection-Based AST." Encyclopedia. Web. 30 March, 2021.
Nanomotion Detection-Based AST
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This entry is adapted from the peer-reviewed paper 10.3390/antibiotics10030287

Rapid antibiotic susceptibility testing (AST) could play a major role in fighting multidrug-resistant bacteria. Recently, it was discovered that all living organisms oscillate in the range of nanometers and that these oscillations, referred to as nanomotion, stop as soon the organism dies. This finding led to the development of rapid AST techniques based on the monitoring of these oscillations upon exposure to antibiotics.

rapid antibiotic susceptibility testing (AST) nanomotion atomic force microscopy (AFM) B. pertussis

1. Introduction

According to a WHO report [1], a post-antibiotic era—in which common infections and minor injuries can kill—is far from being an apocalyptic fantasy but a very real possibility for our century. This is due to the fast emergence of multidrug-resistant microbial pathogens, which is caused by the extensive, sometimes unnecessary use of antimicrobials and the lack of interest of pharma in developing new compounds. The cost of antimicrobial resistance (AMR) is projected to increase significantly as some models predict a rise in global casualties from the present figure of one million to 10 million in 2050 [2]. To combat the rise of AMR, a profound understanding of the mechanisms of microbial infections, the development of new diagnostic tools and new antimicrobials are necessary.

To rationalize the use of large spectrum antimicrobial drugs, it is essential to have a rapid and sensitive detection system that identifies the most appropriate drug to fight a given microorganism immediately at the admission of the patient in a medical center. Current antimicrobial susceptibility testing (AST) technologies mostly rely on microbial culturing and thus replication, which can therefore take up to 1 to 3 days [3][4]. As a result of the diagnostic’s limited speed, accurate treatment, with effective narrow-range antimicrobial agents, is often replaced by the use of broad-spectrum antimicrobials [5][6][7]. The overuse of broad-spectrum antibiotics accelerates the further rise of AMR worldwide [5]. The development of rapid AST technologies is thus important in the battle against AMR. Rapid AST technologies can therefore have a double effect, firstly increasing the survival rate for patients with infections, and secondly, it could potentially extend the lifespan of current narrow-spectrum antimicrobials [8].

2. Current Antimicrobial Susceptibility Testing (AST) Methods

Fighting the threat of multidrug-resistant pathogens requires a multi-disciplinary approach in which rapid AST plays a critical role. The classical method to determine antibiotic susceptibility is the disk diffusion method [3][9][10][11]. This well-established method requires a growth period before the actual disk test is performed, which also is based on further growth during 16 to 20 h. Since some pathogenic bacteria are non-culturable, other methods have to be used. Therefore, new methods that also allow one to perform AST on non-culturable microorganisms in a short time frame [8] are needed. Current AST methods can be divided into phenotypic and molecular tests [12][13][14].

Phenotypic assays monitor the growth of the microorganism in the presence of antibiotics [15]. Classical AST methods are culture-based (Table 1). Since these methods mostly rely on microbial culturing and thus replication, the performance of these tests takes 1 to 3 days [3][4]. Agar dilution assays, i.e., disk diffusion and E-test methods, are flexible and simple methods that are commonly used in clinical microbiology labs (Table 1). They allow one to determine the minimal inhibitory concentration (MIC). A MIC test can also be used using broth dilution assays, where the MIC corresponds to the lowest concentration of antibiotic that completely inhibits bacterial growth and lacks visible turbidity [16]. Broth macrodilution assays have been miniaturized and automated [3]. Several commercial semi-automated or fully automated instruments have been developed, such as the MicroScan WalkAway, Vitek-2, BD Phoenix, Wider System and Sensititre system [3][4][7][17][18][19][20][21][22][23][24][25][26][27]. The time–kill test is a tool for obtaining information on the dynamic interaction between the antimicrobial and the microbial strain [14]. The time–kill curve reveals a time- or concentration-dependent antimicrobial effect and can be used to determine synergism or antagonism between drugs in combinations [28][29][30][31][32]. Optical-based AST methods have been developed to measure the growth rate, such as the “multiplexed automated digital microscopy (MADM)” method [33][34][35] and the oCelloscope [36], as well as to measure morphological changes of single cells upon antibiotic treatment [37] (Table 1). Recently, electrical-based AST methods that are based on impedance, capacitance, resistance and electrochemical measurements, and mechanical-based methods have also been developed (see Table 1 for some examples).

Table 1. Examples of current phenotypic antibiotic susceptibility testing (AST) methods that are classified according to the measuring principle: culture-based, optical-based, electrical-based and mechanical-based AST methods. MIC: minimal inhibitory concentration.

Method Characteristics Reference
Culture-based AST methods
Broth dilution assay Macro- or microdilution of medium–antibiotic solution and growth evaluation based on turbidity or colorimetric differences. [3][4][7][16][17][18][19][20][21][22][23][24][25][26][27]
Disk diffusion Optical analysis of the resulting colony is based on the growth. MIC determination. [3][9][10][11]
Gradient diffusion Similar to the disk diffusion method using a plastic strip. [38]
Time-kill test Reveals a time- or concentration-dependent antimicrobial effect drugs synergism or antagonism. [28][29][30][31][32]
Optical-based AST methods
Optical tracking of cell division Single-cell division tracking associated with large volume imaging. [39]
Multiplexed automated digital microscopy Optical imaging of cells with quantification of growth rates in the presence of antibiotics. [33][34][35]
oCelloscope Estimate the growth of bacterial cells with an optical microscope. [36]
Single-cell morphological analysis (SCMA) Imaging changes of the morphology of single cells upon antibiotic treatment. [37]
Surface plasmon resonance (SPR) A SPR biosensor was used to determine the susceptibility of Staphylococcus aureus clinical isolates. [40]
Electrical-based AST methods
Electric resistance Growth of cells in a microchannel is directly proportional to the measured resistance change. [41]
Impedance-based Fast Antimicrobial Susceptibility Test (IFAST) Changes in biophysical properties of bacteria measured by impedance cytometry. [42]
Electrochemical Measurement of the change in current due to electrochemical reactions. [43][44][45]
Electrical AST (e-AST) Growth of cells is monitored by detecting capacitance change of bacteria bound to 60 aptamer-functionalized capacitance sensors [46]
Mechanical-based AST methods
Asynchronous magnetic bead rotation Detects bacterial growth, based on the rotation of a cluster of magnetic microparticles. [47]

Molecular techniques rely on the determination of a particular fingerprint associated with the resistance to a specific antibiotic [15][48][49] (Table 2). Real-time PCR techniques and specifically constructed DNA microarrays have been developed to detect a spectrum of genes that could be related to resistance to different antibiotics [15][48][50]. Some of these techniques (e.g., the Xpert MTB/RIF assay [51][52][53]) have been commercialized and are characterized by a very high reliability and speed of execution [13]. In the last 10 years, various methods have been developed that are based on matrix-assisted laser desorption ionization time-of-flight mass spectrometry (MALDI-TOF MS) [54]. MALDI-TOF MS allows for the fast identification of the microbial species [55][56][57][58][59][60][61][62][63][64]. The use of MALDI-TOF MS for AST lies in the combination of MALDI TOF MS identification with an established AST method, such as the combination with Vitek-2 [65] or the BD Phoenix system [66][67]. MALDI-TOF MS has also been combined with stable isotope labeling by amino acid in cell culture (SILAC). This MS method can identify the metabolically inactive microorganisms due to the action of the antibiotic [68]. ATP bioluminence assays can provide a fast antibacterial [69][70][71], antimycobacterial [72][73] and antifungal testing [74][75] where the growth is determined based on the ATP quantification. Another molecular marker for growth that has been used is 16S rRNA [76].

Table 2. Molecular AST methods. SILAC: stable isotope labeling by amino acid in cell culture.

Method Characteristics Reference
16S rRNA identification Influence of antibiotic on growth by measurement of 16S rRNA. [76]
ATP bioluminescence ATP quantification as an estimate of the microbial population metabolic activity. [69][70][71][72][73][74]
DNA microarrays DNA microarray using 70mer oligonucleotide. probes to detect resistance genes. [49]
Real-Time PCR Detection of resistance genes. [50][51][52][53]
MALDI-TOF MS and broth dilution Combination of microbial identification with an established AST method. [65][66]
MALDI-TOF MS and SILAC Identification of metabolic inactive microorganisms upon antibiotic treatment. [68]

In this study, we will essentially focus on a novel way to characterize the susceptibility of microorganisms to antibiotics. The technique relies on the detection of the nanometric scale oscillations that characterize living cells. Several years ago, our team demonstrated that all living organisms oscillate at a nanometric scale and that these oscillations end as soon the organism dies [77]. Highlighting such minute movements on a single microorganism requires highly sensitive devices such as atomic force microscopes (AFMs). These instruments are particularly adapted to such challenges, since they can detect displacements in the range of 0.1 Å with a temporal resolution in the range of microseconds. As an illustration, the typical distance between two carbon atoms in an organic molecule is about 2 Å. The very first and straightforward application of such a life monitor is rapid AST. The aim of this article is to describe the working principle of these novel devices, to review their contributions to the field of AST and to discuss their future applications.

3. AFM Nanomotion Setup and Measurement

The technique is relatively simple to set up. A detailed procedure describing the preparation measurement and the data processing steps can be found in Venturelli et al. [78]. Briefly, the first step consists of functionalizing a relatively soft (0.06 N/m) AFM cantilever with a cross linking molecule such as glutaraldehyde, paraformaldehyde, APTES ((3-aminopropyl)triethoxysilane) or fibronectin. To ensure a stronger binding, we recommend a suspension of the microorganism in a phosphate-buffered saline (PBS) solution first. Cell membrane parts, various peptides or amino acids present in traditional culture media can hide the attachment spots on the cross-linking molecules. To ensure the attachment, the cantilever is immersed in a droplet containing the bacteria for about 15 min. The sensor is eventually inserted in the analysis chamber of the AFM to start the measurement. Biologically oriented instruments are preferable since they are designed to operate in liquids and permit one to exchange the “imaging” medium during the measurement. Custom built devices such the one depicted in Figure 1 can also be used.

Antibiotics 10 00287 g003 550

Figure 1. Dedicated nanomotion detection apparatus. 1. analysis chamber with the AFM cantilever, 2. inlet, 3. outlet, 4. laser inlet, 5. prisms to orient the laser beam onto the cantilever and the photodiodes, 6. photodiodes.

The analysis chamber is then filled with the culture medium and the laser beam as well as the two- or four-segment photodiodes are adjusted to achieve the highest possible sensitivity. The measurement usually starts 5–10 min after the insertion of the cantilever into the analysis chamber. This delay permits the liquid medium and the cantilever to reach a thermal steady state. Typical measurements are carried out with a sampling rate of about 20 kHz. Such a high rate is preferred, since it permits one to capture the resonant frequency of the cantilever and to assess the correct position of the laser beam. The oscillations of the lever are recorded for about 15 min in the culture medium before the addition of the antibiotic. Usually, after 10–15 min exposure of bacteria to the drug, the oscillation amplitude drops if the bacteria are sensitive and remains stable or even increases if they are resistant. The experiment can be stopped at this stage; however, we usually inject an additional killing agent such as glutaraldehyde or paraformaldehyde to ensure that the oscillation amplitude drops to zero once all the organisms present on the cantilever are dead.

4. AFM Nanomotion Data Processing

The data processing step consists of a high pass filtering of the original data set to get rid of the thermal drift of the cantilever. The resulting data are eventually processed to extract the variance in a temporal window of 10 s. The variance of the signal is up to now the most sensitive parameter we found to distinguish between living and dead cells. A trial-and-error process in which we attempted to maximize the difference between signals recorded on living and dead samples determined the size of this 10 s window. It is important to mention that the amplitude of the variance signal directly correlates to the nutrient concentrations in the analysis chamber. This observation significantly extends the technique application domains.

Interestingly, frequency domain analysis did not reveal up to now any preferential peak (i.e., frequency) that we could attribute to the specific bacterial species or a metabolic state. However, we noticed that on the fast Fourier transforms (FFT) of the signal, the largest difference between living and dead cells is located between 0.2 and 100 Hz. This frequency window is very stable among all the living organisms that we, and other groups, explored up to now [79].

 

References

  1. WHO. Antimicrobial Resistance: Global Report on Surveillance 2014; World Health Organization: Geneva, Switzerland, 2016.
  2. Michael, C.A.; Dominey-Howes, D.; Labbate, M. The Antimicrobial Resistance Crisis: Causes, Consequences, and Management. Front. Public Heath 2014, 2, 145.
  3. Jorgensen, J.H.; Ferraro, M.J. Antimicrobial Susceptibility Testing: A Review of General Principles and Contemporary Practices. Clin. Infect. Dis. 2009, 49, 1749–1755.
  4. Syal, K.; Mo, M.; Yu, H.; Iriya, R.; Jing, W.; Guodong, S.; Wang, S.; Grys, T.E.; Haydel, S.E.; Tao, N. Current and emerging techniques for antibiotic susceptibility tests. Theranostics 2017, 7, 1795–1805.
  5. Van Boeckel, T.P.; Gandra, S.; Ashok, A.; Caudron, Q.; Grenfell, B.T.; Levin, S.A.; Laxminarayan, R. Global antibiotic consumption 2000 to 2010: An analysis of national pharmaceutical sales data. Lancet Infect. Dis. 2014, 14, 742–750.
  6. Van Boeckel, T.; Laxminarayan, R. Correction to global antibiotic consumption data. Lancet Infect. Dis. 2017, 17, 476–477.
  7. Humphries, R.M.; Hindler, J.A. Emerging Resistance, new antimicrobial agents … but no tests! the challenge of antimicrobial susceptibility testing in the current us regulatory landscape. Clin. Infect. Dis. 2016, 63, 83–88.
  8. Van Belkum, A.; Bachmann, T.T.; Lüdke, G.; Lisby, J.G.; Kahlmeter, G.; Mohess, A.; Becker, K.; Hays, J.P.; Woodford, N.; Mitsakakis, K.; et al. Developmental roadmap for antimicrobial susceptibility testing systems. Nat. Rev. Microbiol. 2019, 17, 51–62.
  9. Horvat, R.T. Review of Antibiogram Preparation and Susceptibility Testing Systems. Hosp. Pharm. 2010, 45, 6–9.
  10. Kronvall, G.; Giske, C.G.; Kahlmeter, G. Setting interpretive breakpoints for antimicrobial susceptibility testing using disk diffusion. Int. J. Antimicrob. Agents 2011, 38, 281–290.
  11. Matuschek, E.; Brown, D.F.J.; Kahlmeter, G. Development of the EUCAST disk diffusion antimicrobial susceptibility testing method and its implementation in routine microbiology laboratories. Clin. Microbiol. Infect. 2014, 20, O255–O266.
  12. Fournier, P.E.; Drancourt, M.; Colson, P.; Rolain, J.M.; La Scola, B.; Raoult, D. Modern clinical microbiology: New challenges and solutions. Nat. Rev. Microbiol. 2013, 11, 574–585.
  13. Dinarelli, S.; Girasole, M.; Kasas, S.; Longo, G. Nanotools and molecular techniques to rapidly identify and fight bacterial infections. J. Microbiol. Methods 2017, 138, 72–81.
  14. Balouiri, M.; Sadiki, M.; Ibnsouda, S.K. Methods for in vitro evaluating antimicrobial activity: A review. J. Pharm. Anal. 2016, 6, 71–79.
  15. Didelot, X.; Bowden, R.; Wilson, D.J.; Peto, T.E.A.; Crook, D.W. Transforming clinical microbiology with bacterial genome sequencing. Nat. Rev. Genet. 2012, 13, 601–612.
  16. Wiegand, I.; Hilpert, K.; Hancock, R.E.W. Agar and broth dilution methods to determine the minimal inhibitory concentration (MIC) of antimicrobial substances. Nat. Protoc. 2008, 3, 163–175.
  17. Lavallée, C.; Rouleau, D.; Gaudreau, C.; Roger, M.; Tsimiklis, C.; Locas, M.C.; Gagnon, S.; Delorme, J.; Labbé, A.C. Performance of an agar dilution method and a Vitek 2 card for detection of inducible clindamycin resistance in Staphylococcus spp. J. Clin. Microbiol. 2010, 48, 1354–1357.
  18. Gardiner, B.J.; Grayson, M.L.; Wood, G.M. Inducible resistance to clindamycin in Staphylococcus aureus: Validation of Vitek-2 against CLSI D-test. Pathology 2013, 45, 181–184.
  19. Tan, Y.E.; Ng, L.S.Y.; Tan, T.Y. Evaluation of Enterococcus faecalis clinical isolates with “penicillin-resistant, ampicillin-susceptible” phenotype as reported by Vitek-2 Compact system. Pathology 2014, 46, 544–550.
  20. Won, E.J.; Shin, J.H.; Kim, M.N.; Choi, M.J.; Joo, M.Y.; Kee, S.J.; Shin, M.G.; Suh, S.P.; Ryang, D.W. Evaluation of the BD Phoenix system for identification of a wide spectrum of clinically important yeast species: A comparison with Vitek 2-YST. Diagn. Microbiol. Infect. Dis. 2014, 79, 477–480.
  21. McGregor, A.; Schio, F.; Beaton, S.; Boulton, V.; Perman, M.; Gilbert, G. The microscan walkaway diagnostic microbiology system—An evaluation. Pathology 1995, 27, 172–176.
  22. Winstanley, T.; Courvalin, P. Expert systems in clinical microbiology. Clin. Microbiol. Rev. 2011, 24, 515–556.
  23. Snyder, J.W.; Munier, G.K.; Johnson, C.L. Direct comparison of the BD phoenix system with the MicroScan WalkAway system for identification and antimicrobial susceptibility testing of Enterobacteriaceae and nonfermentative gram-negative organisms. J. Clin. Microbiol. 2008, 46, 2327–2333.
  24. Mittman, S.A.; Huard, R.C.; Della-Latta, P.; Whittier, S. Comparison of BD Phoenix to Vitek 2, MicroScan MICroSTREP, and Etest for antimicrobial susceptibility testing of Streptococcus pneumoniae. J. Clin. Microbiol. 2009, 47, 3557–3561.
  25. Cantón, R.; Pérez-Vázquez, M.; Oliver, A.; Sánchez Del Saz, B.; Gutiérrez, M.O.; Martínez-Ferrer, M.; Baquero, F. Evaluation of the wider system, a new computer-assisted image-processing device for bacterial identification and susceptibility testing. J. Clin. Microbiol. 2000, 38, 1339–1346.
  26. Swenson, J.M.; Anderson, K.F.; Lonsway, D.R.; Thompson, A.; McAllister, S.K.; Limbago, B.M.; Carey, R.B.; Tenover, F.C.; Patel, J.B. Accuracy of commercial and reference susceptibility testing methods for detecting vancomycin-intermediate Staphylococcus aureus. J. Clin. Microbiol. 2009, 47, 2013–2017.
  27. Junkins, A.D.; Lockhart, S.R.; Heilmann, K.P.; Dohrn, C.L.; Von Stein, D.L.; Winokur, P.L.; Doern, G.V.; Richter, S.S. BD Phoenix and Vitek 2 detection of mecA-mediated resistance in Staphylococcus aureus with cefoxitin. J. Clin. Microbiol. 2009, 47, 2879–2882.
  28. Pfaller, M.A.; Sheehan, D.J.; Rex, J.H. Determination of Fungicidal Activities against Yeasts and Molds: Lessons Learned from Bactericidal Testing and the Need for Standardization. Clin. Microbiol. Rev. 2004, 17, 268–280.
  29. Konaté, K.; Mavoungou, J.F.; Lepengué, A.N.; Aworet-Samseny, R.R.R.; Hilou, A.; Souza, A.; Dicko, M.H.; M’Batchi, B. Antibacterial activity against β- lactamase producing Methicillin and Ampicillin-resistants Staphylococcus aureus: Fractional Inhibitory Concentration Index (FICI) determination. Ann. Clin. Microbiol. Antimicrob. 2012, 11, 1–12.
  30. White, R.L.; Burgess, D.S.; Manduru, M.; Bosso, J.A. Comparison of three different in vitro methods of detecting synergy: Time-kill, checkerboard, and E test. Antimicrob. Agents Chemother. 1996, 40, 1914–1918.
  31. Clancy, C.J.; Huang, H.; Cheng, S.; Derendorf, H.; Nguyen, M.H. Characterizing the effects of caspofungin on Candida albicans, Candida parapsilosis, and Candida glabrata isolates by simultaneous time-kill and postantifungal-effect experiments. Antimicrob. Agents Chemother. 2006, 50, 2569–2572.
  32. Klepser, M.E.; Ernst, E.J.; Lewis, R.E.; Ernst, M.E.; Pfaller, M.A. Influence of test conditions on antifungal time-kill curve results: Proposal for standardized methods. Antimicrob. Agents Chemother. 1998, 42, 1207–1212.
  33. Chantell, C. Multiplexed Automated Digital Microscopy for Rapid Identification and Antimicrobial Susceptibility Testing of Bacteria and Yeast Directly from Clinical Samples. Clin. Microbiol. Newsl. 2015, 37, 161–167.
  34. Price, C.S.; Kon, S.E.; Metzger, S. Rapid antibiotic susceptibility phenotypic characterization of Staphylococcus aureus using automated microscopy of small numbers of cells. J. Microbiol. Methods 2014, 98, 50–58.
  35. Douglas, I.S.; Price, C.S.; Overdier, K.H.; Wolken, R.F.; Metzger, S.W.; Hance, K.R.; Howson, D.C. Rapid automated microscopy for microbiological surveillance of ventilator-associated pneumonia. Am. J. Respir. Crit. Care Med. 2015, 191, 566–573.
  36. Fredborg, M.; Andersen, K.R.; Jørgensen, E.; Droce, A.; Olesen, T.; Jensen, B.B.; Rosenvinge, F.S.; Sondergaard, T.E. Real-time optical antimicrobial susceptibility testing. J. Clin. Microbiol. 2013, 51, 2047–2053.
  37. Choi, J.; Jung, Y.G.; Kim, J.; Kim, S.; Jung, Y.; Na, H.; Kwon, S. Rapid antibiotic susceptibility testing by tracking single cell growth in a microfluidic agarose channel system. Lab Chip 2013, 13, 280–287.
  38. Brown, D.F.J.; Brown, L. Evaluation of the e test, a novel method of quantifying antimicrobial activity. J. Antimicrob. Chemother. 1991, 27, 185–190.
  39. Zhang, F.; Jiang, J.; McBride, M.; Yang, Y.; Mo, M.; Iriya, R.; Peterman, J.; Jing, W.; Grys, T.; Haydel, S.E.; et al. Direct Antimicrobial Susceptibility Testing on Clinical Urine Samples by Optical Tracking of Single Cell Division Events. Small 2020, 16, 2004148.
  40. Tawil, N.; Mouawad, F.; Lévesque, S.; Sacher, E.; Mandeville, R.; Meunier, M. The differential detection of methicillin-resistant, methicillin-susceptible and borderline oxacillin-resistant Staphylococcus aureus by surface plasmon resonance. Biosens. Bioelectron. 2013, 49, 334–340.
  41. Yang, Y.; Gupta, K.; Ekinci, K.L. All-electrical monitoring of bacterial antibiotic susceptibility in a microfluidic device. Proc. Natl. Acad. Sci. USA 2020, 117, 10639–10644.
  42. Spencer, D.C.; Paton, T.F.; Mulroney, K.T.; Inglis, T.J.J.; Sutton, J.M.; Morgan, H. A fast impedance-based antimicrobial susceptibility test. Nat. Commun. 2020, 11, 1–11.
  43. Ertl, P.; Robello, E.; Battaglini, F.; Mikkelsen, S.R. Rapid antibiotic susceptibility testing via electrochemical measurement of ferricyanide reduction by Escherichia coli and Clostridium sporogenes. Anal. Chem. 2000, 72, 4957–4964.
  44. Mann, T.S.; Mikkelsen, S.R. Antibiotic susceptibility testing at a screen-printed carbon electrode array. Anal. Chem. 2008, 80, 843–848.
  45. Onishi, K.; Enomoto, J.; Araki, T.; Takagi, R.; Suzuki, H.; Fukuda, J. Electrochemical microdevices for rapid and on-site determination of the minimum inhibitory concentration of antibiotics. Analyst 2018, 143, 396–399.
  46. Lee, K.S.; Lee, S.M.; Oh, J.; Park, I.H.; Song, J.H.; Han, M.; Yong, D.; Lim, K.J.; Shin, J.S.; Yoo, K.H. Electrical antimicrobial susceptibility testing based on aptamer-functionalized capacitance sensor array for clinical isolates. Sci. Rep. 2020, 10, 1–9.
  47. Kinnunen, P.; McNaughton, B.H.; Albertson, T.; Sinn, I.; Mofakham, S.; Elbez, R.; Newton, D.W.; Hunt, A.; Kopelman, R. Self-assembled magnetic bead biosensor for measuring bacterial growth and antimicrobial susceptibility testing. Small 2012, 8, 2477–2482.
  48. Frye, J.G.; Jesse, T.; Long, F.; Rondeau, G.; Porwollik, S.; McClelland, M.; Jackson, C.R.; Englen, M.; Fedorka-Cray, P.J. DNA microarray detection of antimicrobial resistance genes in diverse bacteria. Int. J. Antimicrob. Agents 2006, 27, 138–151.
  49. Frye, J.G.; Lindsey, R.L.; Rondeau, G.; Porwollik, S.; Long, F.; McClelland, M.; Jackson, C.R.; Englen, M.D.; Meinersmann, R.J.; Berrang, M.E.; et al. Development of a DNA microarray to detect antimicrobial resistance genes identified in the national center for biotechnology information database. Microb. Drug Resist. 2010, 16, 9–19.
  50. Huletsky, A.; Giroux, R.; Rossbach, V.; Gagnon, M.; Vaillancourt, M.; Bernier, M.; Gagnon, F.; Truchon, K.; Bastien, M.; Picard, F.J.; et al. New Real-Time PCR Assay for Rapid Detection of Methicillin-Resistant Staphylococcus aureus Directly from Specimens Containing a Mixture of Staphylococci. J. Clin. Microbiol. 2004, 42, 1875–1884.
  51. Boehme, C.C.; Nabeta, P.; Hillemann, D.; Nicol, M.P.; Shenai, S.; Krapp, F.; Allen, J.; Tahirli, R.; Blakemore, R.; Rustomjee, R.; et al. Rapid Molecular Detection of Tuberculosis and Rifampin Resistance. N. Engl. J. Med. 2010, 363, 1005–1015.
  52. Opota, O.; Mazza-Stalder, J.; Greub, G.; Jaton, K. The rapid molecular test Xpert MTB/RIF ultra: Towards improved tuberculosis diagnosis and rifampicin resistance detection. Clin. Microbiol. Infect. 2019, 25, 1370–1376.
  53. Chakravorty, S.; Simmons, A.M.; Rowneki, M.; Parmar, H.; Cao, Y.; Ryan, J.; Banada, P.P.; Deshpande, S.; Shenai, S.; Gall, A.; et al. The new Xpert MTB/RIF ultra: Improving detection of Mycobacterium tuberculosis and resistance to Rifampin in an assay suitable for point-of-care testing. mBio 2017, 8, e00812-17.
  54. Burckhardt, I.; Zimmermann, S. Susceptibility Testing of Bacteria Using Maldi-Tof Mass Spectrometry. Front. Microbiol. 2018, 9, 1744.
  55. Degand, N.; Carbonnelle, E.; Dauphin, B.; Beretti, J.L.; Le Bourgeois, M.; Sermet-Gaudelus, I.; Segonds, C.; Berche, P.; Nassif, X.; Ferroni, A. Matrix-assisted laser desorption ionization-time of flight mass spectrometry for identification of nonfermenting gram-negative bacilli isolated from cystic fibrosis patients. J. Clin. Microbiol. 2008, 46, 3361–3367.
  56. Seng, P.; Drancourt, M.; Gouriet, F.; La Scola, B.; Fournier, P.E.; Rolain, J.M.; Raoult, D. Ongoing revolution in bacteriology: Routine identification of bacteria by matrix-assisted laser desorption ionization time-of-flight mass spectrometry. Clin. Infect. Dis. 2009, 49, 543–551.
  57. Ledeboer, N.A.; Hodinka, R.L. Molecular detection of resistance determinants. J. Clin. Microbiol. 2011, 49, S20–S24.
  58. Neville, S.A.; LeCordier, A.; Ziochos, H.; Chater, M.J.; Gosbell, I.B.; Maley, M.W.; Van Hal, S.J. Utility of matrix-assisted laser desorption ionization-time of flight mass spectrometry following introduction for routine laboratory bacterial identification. J. Clin. Microbiol. 2011, 49, 2980–2984.
  59. Dubois, D.; Leyssene, D.; Chacornac, J.P.; Kostrzewa, M.; Schmit, P.O.; Talon, R.; Bonnet, R.; Delmas, J. Identification of a variety of Staphylococcus species by matrix-assisted laser desorption ionization-time of flight mass spectrometry. J. Clin. Microbiol. 2010, 48, 941–945.
  60. Saleeb, P.G.; Drake, S.K.; Murray, P.R.; Zelazny, A.M. Identification of mycobacteria in solid-culture media by matrix-assisted laser desorption ionization-time of flight mass spectrometry. J. Clin. Microbiol. 2011, 49, 1790–1794.
  61. Dhiman, N.; Hall, L.; Wohlfiel, S.L.; Buckwalter, S.P.; Wengenack, N.L. Performance and cost analysis of matrix-assisted laser desorption ionization-time of flight mass spectrometry for routine identification of yeast. J. Clin. Microbiol. 2011, 49, 1614–1616.
  62. Croxatto, A.; Prod’hom, G.; Durussel, C.; Greub, G. Preparation of a blood culture pellet for rapid bacterial identification and antibiotic susceptibility testing. J. Vis. Exp. 2014, e51985.
  63. Opota, O.; Croxatto, A.; Prod’hom, G.; Greub, G. Blood culture-based diagnosis of bacteraemia: State of the art. Clin. Microbiol. Infect. 2015, 21, 313–322.
  64. Opota, O.; Jaton, K.; Greub, G. Microbial diagnosis of bloodstream infection: Towards molecular diagnosis directly from blood. Clin. Microbiol. Infect. 2015, 21, 323–331.
  65. Kathuria, S.; Singh, P.K.; Sharma, C.; Prakash, A.; Masih, A.; Kumar, A.; Meis, J.F.; Chowdhary, A. Multidrug-resistant Candida auris misidentified as Candida haemulonii: Characterization by matrix-assisted laser desorption ionization-time of flight mass spectrometry and DNA sequencing and its antifungal susceptibility profile variability by vitek 2, CLSI broth microdilution, and etest method. J. Clin. Microbiol. 2015, 53, 1823–1830.
  66. Hazelton, B.; Thomas, L.C.; Olma, T.; Kok, J.; O′Sullivan, M.; Chen, S.C.A.; Iredell, J.R. Rapid and accurate direct antibiotic susceptibility testing of blood culture broths using MALDI sepsityper combined with the BD phoenix automated system. J. Med. Microbiol. 2014, 63, 1590–1594.
  67. Morgenthaler, N.G.; Kostrzewa, M. Rapid identification of pathogens in positive blood culture of patients with sepsis: Review and meta-analysis of the performance of the Sepsityper kit. Int. J. Microbiol. 2015, 2015, 827416.
  68. Jung, J.S.; Eberl, T.; Sparbier, K.; Lange, C.; Kostrzewa, M.; Schubert, S.; Wieser, A. Rapid detection of antibiotic resistance based on mass spectrometry and stable isotopes. Eur. J. Clin. Microbiol. Infect. Dis. 2014, 33, 949–955.
  69. Finger, S.; Wiegand, C.; Buschmann, H.J.; Hipler, U.C. Antibacterial properties of cyclodextrin-antiseptics-complexes determined by microplate laser nephelometry and ATP bioluminescence assay. Int. J. Pharm. 2013, 452, 188–193.
  70. VOJTEK, L.; DOBES, P.; BUYUKGUZEL, E.; ATOSUO, J.; HYRSL, P. Bioluminescent assay for evaluating antimicrobial activity in insect haemolymph. Eur. J. Entomol. 2014, 111, 335–340.
  71. Ivančić, V.; Mastali, M.; Percy, N.; Gornbein, J.; Babbitt, J.T.; Li, Y.; Landaw, E.M.; Bruckner, D.A.; Churchill, B.M.; Haake, D.A. Rapid antimicrobial susceptibility determination of uropathogens in clinical urine specimens by use of ATP bioluminescence. J. Clin. Microbiol. 2008, 46, 1213–1219.
  72. Andreu, N.; Fletcher, T.; Krishnan, N.; Wiles, S.; Robertson, B.D. Rapid measurement of antituberculosis drug activity in vitro and in macrophages using bioluminescence. J. Antimicrob. Chemother. 2012, 67, 404–414.
  73. Beckers, B.; Lang, H.R.M.; Schimke, D.; Lammers, A. Evaluation of a bioluminescence assay for rapid antimicrobial susceptibility testing of mycobacteria. Eur. J. Clin. Microbiol. 1985, 4, 556–561.
  74. Finger, S.; Wiegand, C.; Buschmann, H.J.; Hipler, U.C. Antimicrobial properties of cyclodextrin-antiseptics-complexes determined by microplate laser nephelometry and ATP bioluminescence assay. Int. J. Pharm. 2012, 436, 851–856.
  75. Galiger, C.; Brock, M.; Jouvion, G.; Savers, A.; Parlato, M.; Ibrahim-Granet, O. Assessment of efficacy of antifungals against Aspergillus fumigatus: Value of real-time bioluminescence imaging. Antimicrob. Agents Chemother. 2013, 57, 3046–3059.
  76. Mach, K.E.; Mohan, R.; Baron, E.J.; Shih, M.-C.; Gau, V.; Wong, P.K.; Liao, J.C. A biosensor platform for rapid antimicrobial susceptibility testing directly from clinical samples. J. Urol. 2011, 185, 148–153.
  77. Longo, G.; Alonso-Sarduy, L.; Rio, L.M.; Bizzini, A.; Trampuz, A.; Notz, J.; Dietler, G.; Kasas, S. Rapid detection of bacterial resistance to antibiotics using AFM cantilevers as nanomechanical sensors. Nat. Nanotechnol. 2013, 8, 522–526.
  78. Venturelli, L.; Kohler, A.C.; Stupar, P.; Villalba, M.I.; Kalauzi, A.; Radotic, K.; Bertacchi, M.; Dinarelli, S.; Girasole, M.; Pešić, M.; et al. A perspective view on the nanomotion detection of living organisms and its features. J. Mol. Recognit. 2020, 33, e2849.
  79. Lissandrello, C.; Inci, F.; Francom, M.; Paul, M.R.; Demirci, U.; Ekinci, K.L. Nanomechanical motion of Escherichia coli adhered to a surface. Appl. Phys. Lett. 2014, 105, 113701.
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