Engineering a SERS Sensing Nanoplatform with Self-Sterilization for Undifferentiated and Rapid Detection of Bacteria

The development of a convenient, sensitive, rapid and self-sterilizing biosensor for microbial detection is important for the prevention and control of foodborne diseases. Herein, we designed a surface-enhanced Raman scattering (SERS) sensing nanoplatform based on a capture–enrichment–enhancement strategy to detect bacteria. The gold−Azo@silver−cetyltrimethylammonium bromide (Au−Azo@Ag−CTAB) SERS nanotags were obtained by optimizing the synthesis process conditions. The results showed that the modification of CTAB enabled the nanotags to bind to different bacteria electrostatically. This SERS sensing nanoplatform was demonstrated to be fast (15 min), accurate and sensitive (limit of detection (LOD): 300 and 400 CFU/mL for E. coli and S. aureus, respectively). Of note, the excellent endogenous antibacterial activity of CTAB allowed the complete inactivation of bacteria after the assay process, thus effectively avoiding secondary contamination.


Introduction
Foodborne illness caused by microorganisms has become a serious public health issue around the globe [1][2][3][4][5][6][7]. Pathogenic bacteria even with a low infectious dose in food and water can cause many serious and even fatal diseases due to their rapid reproductive capacity [8]. Therefore, sensitive and accurate detection of pathogens can be an effective measure for the prevention and control of foodborne diseases. However, traditional bacterial culture methods, polymerase chain reaction (PCR) and enzyme-linked immunosorbent assays (ELISA) often encountered some common problems when used for bacterial detection, including long procedural time, expensive reagents, complex sample preparation and specialized operational skills [9][10][11]. There is thus an urgent need to develop a convenient, rapid, low-cost and sensitive method for microbial detection. In addition, it is crucial to effectively inactivate the bacteria in the sample in a timely manner after the detection process, because the surviving pathogenic bacteria can continue to multiply and may cause additional contamination and pose a serious threat to public health [12,13]. Therefore, it is of significance to develop a biosensor that integrates bacterial detection and microbial elimination to respond to public health emergencies caused by microbes.
In recent years, Au-based SERS spectroscopy has received widespread attention in the detection of pathogenic bacteria because of its high sensitivity, high spectral resolution, rapid acquisition rate and spectral fingerprinting [14][15][16][17][18]. Nevertheless, conventional SERS probes usually employ direct attachment of Raman reporter molecules to the surface of probes [19]. These reporter molecules are unstable in complex environments and even easily separated from the SERS substrates [20]. It is shown that placing the Raman reporter molecules between the core and the shell of the SERS nanotags can not only effectively molecules between the core and the shell of the SERS nanotags can not only effectively prevent its leakage and avoid the interference of the reporter molecules by the complex external environment, but also help to improve the sensitivity of the detection [21,22]. Recently, specific SERS probes with photothermal activity have been developed and used for the quantitative analysis and elimination of specific bacteria [23,24]. However, this type of bacterial inactivation requires the use of an external laser light source, which increases the complexity of the experimental operations. In addition, although specific bacterial recognition elements such as antibodies have good binding affinity for target bacteria [25,26], these probes lack universality and thus it is necessary to redesign and prepare SERS probes for different target bacteria. Therefore, it is desirable to develop universal SERS probes with self-sterilization capability for microbial detection.
Here, we proposed a universal SERS nanotag based on the electrostatic attraction between positively charged CTAB and bacteria (negative charge at physiological pH conditions). To avoid the intrinsic fluorescence interference of conventional Raman reporter molecules (e.g., rhodamine), based on the Azo-enhanced Raman scattering strategy [27,28], Azo with an extended conjugated unit and a highly symmetric molecular structure was selected as a Raman reporter. Azo reporters were modified onto nano Au by Au-S bonding, followed by the growth of Ag shells and surface functionalization with CTAB to obtain Au−Azo@Ag−CTAB nanotags ( Figure 1A). The nanotags were incubated with bacteria for 10 min and the samples were collected in glass capillary for direct detection ( Figure 1B). Benefiting from the aggregation effect induced by the electrostatic interactions [29,30], the nanotags enabled the quantitative detection of E. coli and S. aureus. Furthermore, since CTAB leads to the destruction of the bacterial surface structure, resulting in significant collapse of the bacteria and leakage of the cytoplasm [31,32], the SERS nanotags exhibited excellent intrinsic bactericidal activity, thus avoiding secondary contamination after bacterial detection.

Preparation of Au Nanoparticles (NPs)
Au NPs were synthesized by the classical reduction method of sodium citrate [33]. 100 mL of deionized water was added to a flask washed with aqua regia, lye and deionized water, respectively, and then the flask was heated in an oil bath at 130 • C under stirring (1500 rpm). After boiling, 1 mL of HAuCl 4 solution (0.29 mM) was added and heating continued for 10 min, followed by quick addition of 1.2 mL of sodium citrate solution (38.8 mM). Au NP was obtained after continuing stirring for 30 min. After cooling naturally to room temperature, the Au NP solution was stored in a refrigerator at 4 • C.

Preparation of Au−Azo NPs
A total of 5 mL of the above Au NP solution was added into glass vials, followed by the addition of different volumes of Azo reporter solution (1, 2, 5, 10 and 15 µL, 1mM) pre-dissolved in DMSO, respectively. The mixed solution was stirred (800 rpm) at room temperature for 4 h and then washed three times by centrifugation (3000 rpm, 30 min) using a benchtop centrifuge (TG16-11, Pingfan Instrument & Meter Co. Ltd., Changsha, China). Finally, the different Au−Azo NP solutions were stored in the refrigerator at 4 • C for further use.

Preparation of Au−Azo@Ag NPs
A total of 5 mL of the as-prepared Au−Azo NP solution was added into a flask, and then 200 µL of sodium citrate solution (4.8 mM) was added and the mixed solution was stirred for 5 min (800 rpm), followed by rapid addition of 50 µL of AA solution (0.1 M). Then, different volumes of AgNO 3 solutions (0.01 M, 25, 50, 75, 100 µL) were added into the flasks, respectively. After continuing stirring for 2 h at room temperature, the reaction solution was washed three times by centrifugation (3000 rpm, 30 min) to remove the free Ag ions. Finally, the Au−Azo@Ag NPs were resuspended with deionized water and stored in the refrigerator at 4 • C for further use.

Preparation of Au−Azo@Ag−CTAB NPs
A total of 10 mL of the prepared Au−Azo@Ag NP solution was added into a flask. Then, different volumes of CTAB solutions (0.01 M, 50, 100, 200 µL) were added and the mixed solution was stirred for 5 min (800 rpm). The reaction solution was left to settle overnight at room temperature, followed by washing three times by centrifugation (3000 r/min, 30 min) to remove free CTAB. Finally, the Au−Azo@Ag−CTAB NPs were resuspended with deionized water and stored in the refrigerator at 4 • C.

Ultraviolet-Visible (UV-vis) Spectral Characterization
The UV-vis absorbance of the product in each step was recorded using a UV-3600 spectrophotometer (Shimadzu). UV-vis spectroscopic characterization provides a reference for NP stability. The UV-vis spectra were obtained as follows: after baseline calibration, the sample solution was added to the cuvette and then scanned in the selected wavelength range (300-800 nm).

Dynamic Light Scattering (DLS) and Zeta Potential Characterization
The hydrated size and zeta potential of NPs were determined by using the Malvern particle sizer (ZS90, Malvern). The DLS characterization showed the size distribution of NPs, while the zeta potential characterization showed the surface electrical properties of NPs. The details are as follows: the NP solution was added to a specific sample cell (size: DTS0012, potential: DTS1070) and then the sample solution was subsequently detected by the corresponding mode.

Field Emission Scanning Electron Microscopy (FE-SEM) Characterization
The morphology of NPs, Au−Azo@Ag−CTAB anchored E. coli and Au−Azo@Ag− CTAB anchored S. aureus was characterized by FE-SEM (Zeiss SIGMA, Carl Zeiss AG, Jena, Germany). The specific experimental method was as follows: the appropriate concentration of sample solution was dropped onto a conductive single-crystal silicon wafer. After drying naturally, the samples sprayed with gold were characterized morphologically using an Inlens detector. The test voltage was 10 KV.

Raman Spectroscopy Characterization
To optimize the addition volume of Azo reporters, Ag ions and CTAB, the Au−Azo NPs, Au−Azo@Ag NPs and Au−Azo@Ag−CTAB NPs were characterized by Raman spectroscopy (InVia, Renishaw, Wotton-under-Edge, UK), respectively. The experimental procedure was as follows: a certain volume of sample solution was aspirated with a glass capillary tube (5 mm diameter), and then the capillary tube was placed under a microscope (20× objective) and the sample stage was adjusted so that the capillary tube was in focus under the laser, followed by Raman signal acquisition. Acquisition conditions: excitation wavelength of 633 nm, laser power of 10 mW, integration time of 1 s, and accumulation of 1 time. The Raman spectra were acquired in the spectral range from 950 to 1620 cm −1 . The initial Raman spectrum in this study was calibrated and smoothed by WIRE 3.4 software (intelligent fitting, polynomial order of 10, noise tolerance of 1.50), and the peak intensity at 1120 cm −1 (Ph-N) was used for quantitative analysis [28].

Bacterial Culture
The lyophilized powder of E. coli (ATCC 8099) and S. aureus (ATCC 25923) was transferred into LB liquid medium (5 mL) respectively, followed by incubation (37 • C, 200 rpm) in a constant temperature shaking incubator (PTQZ-6, Changzhou Putian Instrument Manufacturing Co., Ltd., Changzhou, China) until the bacterial concentration reached 1 × 10 8 CFU/mL. Afterward, the two bacteria solutions were collected by centrifugation (3000 rpm, 10 min) and washed with PBS three times. Prior to the test of the bacterial sample, the concentrations of bacteria suspended in PBS were determined by spread plate method.

Bacterial Quantification Using Au−Azo@Ag−CTAB NPs
The two bacterial solutions (S. aureus and E. coli) were diluted separately with PBS to a concentration of 1 × 10 7 CFU/mL according to the results of plate counting. Then the diluted bacterial solution was used as mother liquor to prepare four groups of bacterial solutions with different concentrations (1 × 10 6 CFU/mL, 1 × 10 5 CFU/mL, 1 × 10 4 CFU/mL and 1 × 10 3 CFU/mL). Afterwards, 20 µL of Au−Azo@Ag−CTAB NP solution was added to 200 µL of different concentrations of bacterial solution, respectively. The mixture was shaken for 10 min and then aspirated with a capillary tube and placed under a microscope (10× objective, NA = 0.4) for Raman spectroscopy. The test conditions were the same as described in Section 2.9.

Bacterial Detection and Inactivation in Tap Water
The S. aureus and E. coli with unknown concentrations were added to the tap water and shaken thoroughly for 10 min, respectively. Then 100 µL of the above bacterial solution was blended with 20 µL of Au−Azo@Ag−CTAB NP solution. The Raman spectra were acquired according to the method constructed in Section 2.11. The accuracy of our method in detecting bacteria in real samples was evaluated by comparing it with the culturing results. To verify the antibacterial ability of Au−Azo@Ag−CTAB nanotags, the bacteria/Au−Azo@Ag−CTAB nanotag mixture was plated on a solid LB medium and incubated for 24 h at 37 • C, followed by counting the number of the bacterial colonies. The bacteria without any treatment were acted as control.

Synthesis and Characterization of Au−Azo@Ag−CTAB NPs
During the preparation of the Au−Azo@Ag−CTAB NPs, the addition amount of the Azo signal molecules, AgNO 3 and CTAB has an important impact on the SERS signal strength and stability of the NPs, and thus it is necessary to optimize these parameters.

Optimization of Synthesis Conditions of Au NPs
The Au NPs were first prepared by the classical sodium citrate reduction. It has been reported that the SERS enhancement effect of the Au NPs was related to its size [34]. When the size of the Au NPs increased, the collective oscillation amplitude of free electrons on its surface decreased and the absorption band of surface plasmon resonance broadened, leading to a weaker SERS enhancement effect. However, the SERS enhancement effect was also weak for the small-sized nano Au because of the low light absorption cross section and the low number of excited electrons on the surface. Combining the above factors, the Au NPs with a size of 45 nm were successfully prepared ( Figure 2A). The S. aureus and E. coli with unknown concentrations were added to the tap water and shaken thoroughly for 10 min, respectively. Then 100 µL of the above bacterial solution was blended with 20 µL of Au−Azo@Ag−CTAB NP solution. The Raman spectra were acquired according to the method constructed in Section 2.11. The accuracy of our method in detecting bacteria in real samples was evaluated by comparing it with the culturing results. To verify the antibacterial ability of Au−Azo@Ag−CTAB nanotags, the bacteria/Au−Azo@Ag−CTAB nanotag mixture was plated on a solid LB medium and incubated for 24 h at 37 °C, followed by counting the number of the bacterial colonies. The bacteria without any treatment were acted as control.

Synthesis and Characterization of Au−Azo@Ag−CTAB NPs
During the preparation of the Au−Azo@Ag−CTAB NPs, the addition amount of the Azo signal molecules, AgNO3 and CTAB has an important impact on the SERS signal strength and stability of the NPs, and thus it is necessary to optimize these parameters.

Optimization of Synthesis Conditions of Au NPs
The Au NPs were first prepared by the classical sodium citrate reduction. It has been reported that the SERS enhancement effect of the Au NPs was related to its size [34]. When the size of the Au NPs increased, the collective oscillation amplitude of free electrons on its surface decreased and the absorption band of surface plasmon resonance broadened, leading to a weaker SERS enhancement effect. However, the SERS enhancement effect was also weak for the small-sized nano Au because of the low light absorption cross section and the low number of excited electrons on the surface. Combining the above factors, the Au NPs with a size of 45 nm were successfully prepared (Figure 2A).

Optimization of Synthesis Conditions of Au−Azo NPs
Azo reporters can be modified onto the nano Au through Au-S bonds. The addition volume of Azo reporters was optimized, and the products were marked as Au−Azo−1 to Au−Azo−5 in the order of volume from small to large. The UV-vis spectrum of each product is shown in Figure S2A. With the increase in the addition volume of Azo reporters, the peak intensity of the product at 520 nm gradually reduced, in which the Au−Azo−5 NP solution showed significant sedimentation (as shown in the inset), indicating that the stability of the NPs decreased gradually. In addition, the products were further characterized by Raman spectroscopy. As shown in Figure S2B, compared with other NPs, Au−Azo−4 showed the best SERS enhancement effect, in which the Raman signal at 1120 cm −1 can be attributed to the stretching vibration of the Ph-N bond in Azo. However, the Au−Azo−4 NPs presented an obvious UV-vis absorption peak near 700 nm, which indicated a certain degree of aggregation of the NPs. Collectively, the Au−Azo−3 NPs were selected for subsequent experiments.

Optimization of Synthesis Conditions of Au−Azo@Ag NPs
Similarly, the addition volume of AgNO 3 was optimized and the products were labeled as Au−Azo@Ag−1 to Au−Azo@Ag−4. As shown in Figure S3A, with the increase in the addition volume of AgNO 3 , the UV-vis absorption peak of the Au−Azo@Ag NPs was gradually blue-shifted. The Au−Azo@Ag−3/−4 NP solution presented an obvious absorption peak at 620 nm, and the color of the solution was turbid (as shown in the inset), indicating a certain degree of aggregation of the NPs. In addition, the products were also characterized by Raman spectroscopy ( Figure S3B). Based on the stability and SERS enhancement effect of the Au−Azo@Ag NPs, the Au−Azo@Ag−2 NPs were selected for subsequent experiments.

Optimization of Synthesis Conditions of Au−Azo@Ag−CTAB NPs
The addition volume of CTAB was optimized and the products were labeled as Au−Azo@Ag−CTAB−1 to Au−Azo@Ag−CTAB−3. Because the surface of the Au−Azo@Ag NPs presented a negative charge, CTAB with a positive charge can be modified to the surface of the Au−Azo@Ag NPs by electrostatic action. Figure S4 showed the UV-vis spectra of the Au−Azo@Ag−CTAB NPs with different surface charge densities. With the increase in the CTAB addition volume, the Au−Azo@Ag−CTAB NPs presented a weaker absorption peak at 700 nm, indicating better dispersion stability. The Au−Azo@Ag−CTAB−3 NPs were selected as the optimal SERS nanotags. For the convenience of naming and description, it was uniformly called the Au−Azo@Ag−CTAB NPs in the subsequent experiment.

Characterization of Au−Azo@Ag−CTAB NPs
The Au−Azo@Ag−CTAB NPs with a size of about 55 nm were successfully synthesized step-by-step ( Figure 2B). The results of the EDS-mapping also demonstrated the successful synthesis of the Au−Azo@Ag−CTAB NPs ( Figure 2C). In addition, the hydrated size of the Au−Azo@Ag NPs was significantly larger than the Au NPs, indicating the successful growth of the Ag shells onto the nano Au ( Figure 2D). The results from zeta potential characterization demonstrated that the CTAB (positive charge) was successfully modified on the surface of the Au−Azo@Ag NPs ( Figure 2E). The UV-vis spectrum of each product is shown in Figure 2F. The blue shift of the absorption peak wavelength of the Au−Azo@Ag NPs with respect to the Au NPs indicated the successful formation of the Ag shells.

Ability of Au−Azo@Ag−CTAB NPs to Capture, Detect and Inactivate Bacteria
After mixing the positively charged Au−Azo@Ag−CTAB NPs with bacteria (S. aureus or E. coli), the bacteria can induce the aggregation of the NPs through electrostatic effect, thereby enhancing the SERS signal of the detection system [35]. In order to verify the detection mechanism of this study, the combination of nanotags and bacteria was characterized by SEM. As shown in Figure 3A,B, a large number of NPs were anchored onto the surface of E. coli and S. aureus, respectively, and the density of the nanotags on the surface of E. coli was slightly higher than that of S. aureus, which may be due to the relatively lower surface potential of E. coli ( Figure 3C,D). tection mechanism of this study, the combination of nanotags and bacteria was ch ized by SEM. As shown in Figure 3A,B, a large number of NPs were anchored o surface of E. coli and S. aureus, respectively, and the density of the nanotags on the of E. coli was slightly higher than that of S. aureus, which may be due to the re lower surface potential of E. coli ( Figure 3C,D). To investigate the feasibility of this method for bacterial quantification analy ferent concentrations of E. coli and S. aureus were mixed with the Au−Azo@Ag NPs, respectively, and then determined by Raman spectroscopy. As shown in Fig within the concentration range from 10 3 to 10 7 CFU/mL, the Raman intensity at 11 gradually enhanced with the increase in E. coli concentration. There was a good relationship between the Raman intensity and the logarithm of bacterial concen ( Figure 4B), and the calibration curve for E. coli was y = 1082.9x − 2132 with R 2 of achieving LOD as low as 300 CFU/mL (3 times signal/background). In addition, t tionship between the Raman intensity and the logarithm of the bacterial concen was further explored using S. aureus as a model. Similar to E. coli, there was a p correlation between them ( Figure 4C), and the linear fitting equation was y = 951.4x with R 2 = 0.9834 ( Figure 4D) (LOD: 400 CFU/mL). The results indicated that the intensity of the nanotags prepared in this work had a good linear correlation w logarithm of the concentration of E. coli and S. aureus, respectively. In order to av perimental errors, five randomly selected positions of the capillary tube containing ent concentrations of bacteria/nanotags mixture were tested by Raman spectrosco the results showed the reliability of the method (Figures S5 and S6). To investigate the feasibility of this method for bacterial quantification analysis, different concentrations of E. coli and S. aureus were mixed with the Au−Azo@Ag−CTAB NPs, respectively, and then determined by Raman spectroscopy. As shown in Figure 4A, within the concentration range from 10 3 to 10 7 CFU/mL, the Raman intensity at 1120 cm −1 gradually enhanced with the increase in E. coli concentration. There was a good linear relationship between the Raman intensity and the logarithm of bacterial concentration ( Figure 4B), and the calibration curve for E. coli was y = 1082.9x − 2132 with R 2 of 0.9816, achieving LOD as low as 300 CFU/mL (3 times signal/background). In addition, the relationship between the Raman intensity and the logarithm of the bacterial concentration was further explored using S. aureus as a model. Similar to E. coli, there was a positive correlation between them ( Figure 4C), and the linear fitting equation was y = 951.4x − 1898 with R 2 = 0.9834 ( Figure 4D) (LOD: 400 CFU/mL). The results indicated that the Raman intensity of the nanotags prepared in this work had a good linear correlation with the logarithm of the concentration of E. coli and S. aureus, respectively. In order to avoid experimental errors, five randomly selected positions of the capillary tube containing different concentrations of bacteria/nanotags mixture were tested by Raman spectroscopy, and the results showed the reliability of the method (Figures S5 and S6).
The Au−Azo@Ag−CTAB NPs were expected to possess excellent antibacterial ability due to the ability of CTAB to disrupt the cell surface structure [31]. To verify the bactericidal performance of the Au−Azo@Ag−CTAB NPs, high concentrations (10 7 CFU/mL) of bacteria (S. aureus and E. coli) were incubated with nanotags for 2 h, and then characterized by the spread plate method. As shown in Figure S7, the control group (without treatment) presented a large number of bacterial colonies, while no colonies of E. coli or S. aureus were observed in the Au−Azo@Ag−CTAB NPs group, demonstrating its good antimicrobial activity. Thus, the nanotags had the potential to prevent the secondary contamination of bacteria after detection.  The Au−Azo@Ag−CTAB NPs were expected to possess excellent antibacteria due to the ability of CTAB to disrupt the cell surface structure [31]. To verify the cidal performance of the Au−Azo@Ag−CTAB NPs, high concentrations (10 7 CFU bacteria (S. aureus and E. coli) were incubated with nanotags for 2 h, and then ch ized by the spread plate method. As shown in Figure S7, the control group (witho ment) presented a large number of bacterial colonies, while no colonies of E. c aureus were observed in the Au−Azo@Ag−CTAB NPs group, demonstrating its g timicrobial activity. Thus, the nanotags had the potential to prevent the seconda tamination of bacteria after detection.

Quantitative Detection and Inactivation of Bacteria in Tap Water
Due to the increasing popularity of tap water and its use as the main source o ing water, the detection of microorganisms in tap water is the key to ensure the s drinking water. In order to verify the feasibility of this method in the detection of in tap water, the method of spiked bacteria in tap water was employed. Six gr bacterial sample solutions with unknown concentrations (S. aureus and E. coli) wer with the Au−Azo@Ag−CTAB nanotags, respectively, and then characterized by spectroscopy under the same conditions as stated before. The bacterial concentrat calculated according to the calibration curve of the corresponding bacteria, respe As shown in Table 1, the concentrations of the E. coli and S. aureus detected by our were comparable to that of the standard culture counting with the relative recove ing from 106% to 110%, which indicated that this method was suitable for the dete microorganisms in tap water. The errors may be due to the interference from p impurities such as particulate matters and ionic materials. Furthermore, the detec centration of bacteria was relatively consistent for the repeated measurements w RSD% less than 5%, demonstrating the reliability of our method for tap water mon

Quantitative Detection and Inactivation of Bacteria in Tap Water
Due to the increasing popularity of tap water and its use as the main source of drinking water, the detection of microorganisms in tap water is the key to ensure the safety of drinking water. In order to verify the feasibility of this method in the detection of bacteria in tap water, the method of spiked bacteria in tap water was employed. Six groups of bacterial sample solutions with unknown concentrations (S. aureus and E. coli) were mixed with the Au−Azo@Ag−CTAB nanotags, respectively, and then characterized by Raman spectroscopy under the same conditions as stated before. The bacterial concentration was calculated according to the calibration curve of the corresponding bacteria, respectively. As shown in Table 1, the concentrations of the E. coli and S. aureus detected by our method were comparable to that of the standard culture counting with the relative recovery ranging from 106% to 110%, which indicated that this method was suitable for the detection of microorganisms in tap water. The errors may be due to the interference from potential impurities such as particulate matters and ionic materials. Furthermore, the detected concentration of bacteria was relatively consistent for the repeated measurements with the RSD% less than 5%, demonstrating the reliability of our method for tap water monitoring. Compared to the time-consuming bacterial culture (2-3 days), the whole process of our method can be completed within 15 min, indicating the potential of point-of-care testing (POCT) in bacterial detection. The inactivation ability of the Au−Azo@Ag−CTAB nanotags to bacteria in tap water was characterized by the spread plate method. As shown in Figure 5, no bacterial colonies were found in the Au−Azo@Ag−CTAB nanotags group, which indicated that the bacteria in the tested solution have been completely inactivated, thus effectively avoiding environmental pollution. 5, no bacterial colonies were found in the Au−Azo@Ag−CTAB nanotags group, which dicated that the bacteria in the tested solution have been completely inactivated, thus fectively avoiding environmental pollution.

Conclusions and Future Perspective
In this work, we designed a novel SERS sensing nanoplatform that integrated bro spectrum bacterial detection and self-sterilization. The Au−Azo@Ag−CTAB nanot were prepared based on the rational configuration of the recognition unit, Raman repo and SERS substrate. The positively charged Au−Azo@Ag−CTAB nanotags were ancho on the surface of bacteria through electrostatic action so as to induce the enhancemen

Conclusions and Future Perspective
In this work, we designed a novel SERS sensing nanoplatform that integrated broadspectrum bacterial detection and self-sterilization. The Au−Azo@Ag−CTAB nanotags were prepared based on the rational configuration of the recognition unit, Raman reporter and SERS substrate. The positively charged Au−Azo@Ag−CTAB nanotags were anchored on the surface of bacteria through electrostatic action so as to induce the enhancement of the SERS signal. The results showed that the proposed SERS sensing nanoplatform was sensitive, rapid and reliable for bacterial detection. The recoveries of E. coli ranged from 108% to 110%, and the recoveries of S. aureus ranged from 106% to 107%, both of which demonstrated the feasibility of this method for the quantification of bacteria in tap water. Furthermore, the microorganisms in the tested solution can be killed completely and timely without any treatment, avoiding bacteria contamination after the bacterial detection. The anti-interference capability of the biosensor, which binds bacteria by electrostatic interaction, may need further improvement. Therefore, in the future, we plan to modify the nanotags with mercaptophenylboronic acid to enhance the recognition of bacteria. This SERS sensing nanoplatform has potential applications in the POCT of medical and environmental samples for which rapid in situ testing is required.  Figure S1: The molecular structure of Azo Raman reporter; Figure S2:

Institutional Review Board Statement: Not applicable.
Informed Consent Statement: Not applicable.

Data Availability Statement:
The data presented in this study are available on request from the corresponding author.