Hanhao
Zhang
a,
Divya
Bhakta
a,
Anushka
Saha
a,
Sai Preetham
Peddireddy
a,
Shumin
Bao
b,
Lei
Li
b,
Sukwan
Handali
c,
W. Evan
Secor
c,
Lucia A. O.
Fraga
d,
Jessica K.
Fairley
e and
Aniruddh
Sarkar
*a
aDepartment of Biomedical Engineering, Georgia Institute of Technology, 315 Ferst Dr NW, Atlanta, GA 30332, USA. E-mail: aniruddh.sarkar@bme.gatech.edu
bDepartment of Chemistry and Center for Diagnostics & Therapeutics, Georgia State University, Atlanta, GA 30303, USA
cDivision of Parasitic Diseases and Malaria, National Center for Emerging and Zoonotic Infectious Diseases, Centers for Disease Control and Prevention, Atlanta, GA 30333, USA
dFederal University of Juiz de Fora, Juiz de Fora, Minas Gerais 36036-900, Brazil
eDepartment of Medicine, Division of Infectious Diseases, Emory University School of Medicine, Atlanta, GA 30307, USA
First published on 1st April 2025
Control of endemic infectious diseases is often impeded by the lack of sensitive and specific yet easy-to-obtain biomarkers. Antibody fragment crystallizable (Fc) regions, such as Fc glycosylation, which are modulated in a pathogen-specific and disease-state-specific manner have emerged as potential such biomarkers. However current methods to perform large-scale antigen-specific antibody Fc feature screening for biomarker discovery often require too much sample volume, cost and expertise to be realistically realizable in many disease contexts. Here we present a simple, flexible and reconfigurable microfluidic device, made using rapid prototyping techniques, that can perform highly multiplexed and high-throughput biomarker discovery targeting both antibody fragment antigen-binding (Fab) and Fc features including antigen specificity, antibody isotypes, subclasses, N-glycosylation and Fc receptor binding. Using integration of an antigen microarray and reconfigurable microfluidics for sample and probe distribution, the device can perform a total of 1400 assays measuring 100 antibody Fab and Fc features per sample from a low sample volume (15 μL). The device demonstrates cleanroom-free simple fabrication and ease of use comparable to standard immunoassay platforms. Performance comparable to existing methods was validated and a biomarker screening for schistosomiasis, a helminth-mediated infection, was performed using clinical samples where antibody subclass-based biomarkers were successfully identified distinguishing current infection from former infection and endemic controls.
Direct pathogen detection via microscopy or pathogen-derived molecular biomarker-based tests remains the gold standard but is complex and costly or has low sensitivity for many infections. This can be due to low target abundance, complex sample acquisition (e.g. sputum for TB) and preparation or varying pathogen burden and sequestration in tissue over its life cycle. Monitoring of host immunity, especially antibodies (Abs), can provide an amplified readout of infection. Abs make up to 20% of protein in blood.4 Their abundance in blood and other easily accessible samples, along with their inherent ability to bind pathogen-specific antigens, enables easy testing of their presence using inexpensive formats such as lateral flow assays from small sample volumes.
Ab titer-based tests however cannot accurately distinguish current from past infection and thus have low specificity for endemic infections because Abs tend to linger after infection.5 Abs are composed of two functional domains: fragment antigen-binding (Fab) and fragment crystallizable (Fc) (Fig. 1A). While pathogen-specific binding occurs via the Fab region, effector functions are directed by the Fc region. This Fc region is rapidly modified during an immune response in two distinct ways: a) distinct isotypes (IgG, IgA, IgM, IgE) or subclasses (IgG1–4, IgA1–2) may be selected (Fig. 1B) or b) differential Fc glycosylation may occur, which is a post-translational modification carried by all human Abs (Fig. 1B). Both these Fc modifications regulate Ab binding to complement and Fc receptors carried by immune cells thus regulating host immune functions including antibody-dependent cellular cytotoxicity, phagocytosis, etc.6,7 Among these two, Ab glycosylation has been shown to shift in a disease-state-specific manner7 and thus has emerged as a disease-state-specific predictive biomarker. We have recently shown that a comprehensive measurement of Fab and Fc properties of Abs via antigen specificity, isotype, subtype, glycosylation and Fc receptor binding measurement, coupled to machine-learning-based analytics (termed together as Ab-omics), can be used to predict outcome in severe COVID-19 and disease state in schistosomiasis.8,9 Others have described Ab glycosylation and Fc-related biomarkers in HIV,10 dengue,11 TB,12 rheumatoid arthritis,13 colorectal cancer14 and even aging.15
However, despite increasing interest in Ab glycosylation- and Fc-based biomarkers, there is a scarcity of tools for their discovery from low-volume clinical samples. Mass spectrometry (MS)-based methods remain the gold standard for glycomics studies. However, these are cumbersome, expensive and, critically, require prior isolation of antigen-specific Abs, which demands large volumes of sample (e.g. ∼0.1–1 mL of blood per antigen specificity). Thus, they need an impractically large sample volume for profiling large numbers of antigen-specific Abs (e.g. for a complete immunoproteomic scan of ∼4000 antigens of M. tuberculosis, it would need ∼400–4000 mL of blood per patient). Recently developed glycan-specific probe binding-based methods including lectin-8,9 and nanobody-based Ab glycoprofiling11 and multiplexed Ab Fc profiling methods16,17 offer an opportunity for reducing the sample requirement for Ab Fc biomarker discovery. However, these assays remain too specialized currently compared to standard immunoassays commonplace in clinical research laboratories, such as plate-based enzyme-linked immunosorbent assays (ELISAs). Conversely, traditional ELISAs lack multiplexing ability and would require multiple runs for measuring Fab (antigen) and Fc (probe) combinations adding to labor and sample requirement.
Microfluidics offers an attractive alternative for massively multiplexed immunoassays. Microfluidic devices can test high numbers of samples simultaneously while using only a few microliters from each.18,19 However, fabrication and use of such devices are still complex, requiring techniques and training not easily accessible to clinical research labs with most interest in biomarker discovery, especially in resource-poor settings, which may however be well-trained in typical immunoassay workflows.
To overcome the above obstacles, in this work, we set out to develop a simple, easy-to-manufacture and easy-to-use microscale device that can be used for highly multiplexed Ab Fab and Fc profiling for biomarker discovery from small volumes of clinical samples. We achieved this via the integration of antigen microarrays on glass slides with flexible and reconfigurable microchannels made using widely available rapid prototyping tools. The device and workflow (Fig. 2) are designed to be usable with high tolerance during assembly and operation and with minimal additional training beyond that for a typical multi-channel pipette compatible immunoassay workflow. Here we report the design and development of this chip, which we term as the Microfluidic Multiplexed Antibody-omic Profiling (or μMAP) chip, which performs 1400 Ab Fab and Fc assays simultaneously, establish its performance compared to other methods, and demonstrate its use in characterizing small volumes (15 μL) of clinical samples from schistosomiasis patients to find an active infection-specific biomarker which clearly distinguishes current infection from former infections.
To further simplify the fabrication, we avoid here the conventional process of creating a lithography-based mold and then molding a piece of PDMS. Instead, we formed the enclosed microfluidic channels by simply pressing two pieces of the above thin laser-cut PDMS sheets onto a glass slide. The glass slide serves as the bottom, the middle PDMS sheet, which has laser-cut channels, serves as the side walls while the top PDMS sheet serves as the cover. The PDMS sheet used is commercially available, as a roll, at a low cost (<$20 per sq. ft.). The cutting of the channels only requires simple laser cutting using a basic laser cutter available in most rapid prototyping facilities globally.23 Due to its minimal thickness, the sheet is highly conformable and ensures good sealing when simply pressed against the glass slide. As a result, the fabrication of this microfluidic device does not involve any conventional cleanroom fabrication techniques and can easily be done in a typical wet lab environment. To reduce sample usage by decreasing the height of the channels, 0.01′′ thin PDMS was chosen for the middle sample channel layer. After full assembly, less than 15 μL of sample is enough to fill each vertical sample channel and covers four 25-plex antigen array blocks per column, which equals testing against all combinations of 25 capture antigens and 4 Fc probes – thus measuring a total of 100 Fab and Fc properties per sample. This can be compared to the assay volume of a standard microtiter-plate well in a single-plex ELISA, which is ∼40 μL per feature measured and would thus add to ∼4 mL per sample for the 100 measurements.
The complete μMAP-based assay procedure is shown in Fig. 2. First, the glass slide is spotted with capture antigens in a 5 × 5 array format (see Experimental section for spotting details). 8 different proteins with 3 replicates plus a control are shown in the example array here, yet the type and numbers of antigens are customizable at this stage. Here, each slide has 14 columns and 4 rows of the 5 × 5 antigen array blocks printed. To perform the biomarker discovery experiment, two layers of PDMS are pressed on the glass slide without irreversible bonding to form channels. Samples are then added into the vertical sample channels using a single-channel or multi-channel pipette. These channels get filled by a combination of capillary action and the gravity head due to the sample drop placed at the channel inlet; thus the assay procedure does not require the use of any additional pumping equipment. After sample incubation, these PDMS layers are removed in PBS without cross contamination. The slide is washed and dried, and another two layers of PDMS are attached and four fluorescently labelled Fc probes are added into the 4 horizontal channels for incubation. After PDMS removal and slide washing, a fluorescent signal from each protein dot can be read. Here we use a standard microarray scanner for this as this offers automation in reading, but a standard fluorescence microscope can also be used for this.
To ensure good repeatability, we explored methods to improve the morphology of the printed protein dots. Besides optimizing settings of the printer, we added glycerol as it is known as an agent that can stabilize a liquid drop during protein microarray printing.24 An increase in repeatability of morphology of printed dots was observed by adding more glycerol (Fig. 4D), yet it came at the cost of lower MFI. By considering MFI (Fig. 4E) and variation (Fig. 4F) of the drops, 5% glycerol was chosen as the optimal concentration to achieve a balance. To demonstrate the ability of the device to perform a sandwich binding immunoassay, serial dilutions of monoclonal IgG targeting different antigens were added to different channels of the same chip printed with SARS-CoV-2 antigens. For the channel infused with anti-spike (S) Ab, MFI from both spike and spike RBD (S RBD) protein (which is the receptor binding domain and hence part of the S protein as well) formed a sample dilution-dependent response curve, while MFI from the non-target nucleocapsid (N) protein remained low around background (Fig. 4G), proving the ability to measure the concentration of antibody in buffer quantitatively and specifically. LOD for the above application reached 1 ng mL−1 (6.7 pM), while a dynamic range of >3 orders of magnitude were achieved. Note that this is similar sensitivity to that achieved in typical plate-based single-plex ELISAs. However, it represents higher dynamic range (>3 orders of magnitude) than most plate-based ELISAs (2–3 orders of magnitude) while being multiplexable as well. Similarly, for the channel with anti-N Ab as sample, MFI from N protein spots formed a sample dilution-dependent response curve, while the MFIs from S and S RBD proteins in this channel remained low (Fig. 4H), again verifying the specificity of the immunoassay in the μMAP chip. As the two types of antibodies and probes were all placed in neighboring channels, no cross contamination was again verified. Verification with clinical samples was also performed with serum from a SARS-CoV-2 patient and vaccinated and pre-pandemic healthy individuals. Antigen-specific IgG against 8 antigens were measured using one chip simultaneously. Decreasing MFI of spike-specific antibody when serum dilution increased verified the ability of μMAP to measure antibody titer (Fig. S4†). The measured MFI of IgG against N/S/S RBD between the three groups verified the function and throughput of the μMAP chip (Fig. S5†).
Using serum samples that underwent the above modifications, 100% S and 0% S samples, and mixtures thereof, were tested on the μMAP chip using protein L as the capture antigen spot, which bind all isotypes and subtypes of antibodies via their Fab region. A linear relationship between percentage of sialic acid in samples, measured using LC-MS, and corresponding measured MFI of SNA binding on antibodies on the μMAP chip was observed (Fig. 5C). The linear pattern, repeatability and the high correlation of 0.99 with the gold standard MS indicated that the μMAP chip could accurately quantify the level of sialic acid on antibodies in human serum. One trade-off we observed was that unlike results from LC-MS, the 0% S sample returned an MFI close to that of the 25% S sample. This was likely due to the nature of the lectin probe exhibiting high background binding, and 0% S was out of the dynamic range of this method when used for quantifying glycosylation. Data from the μMAP chip were also highly correlated with data from a bead-based lectin-binding assay (Luminex) with the same set of samples (Fig. 5D). Here, the same issue with measuring 0% S occurred for the bead-based assay, indicating this issue was common to binding assays utilizing this lectin probe and not dependent on the use of the μMAP chip.
Next, we tested if the μMAP chip can simultaneously measure antibody glycosylation of multiple antigen-specific antibodies, which is the key bottleneck in MS-based glycomics that drives high sample usage. Enabled by the high-throughput nature of the chip, sera from healthy individuals containing either unmodified antibodies or asialated/agalactosylated antibodies after in vitro enzymatic glycoengineering of serum as described above were tested against 4 antigens (Protein L, CMV pp65, Tetanus (TTA), and SARS-CoV-2 nsp13) and 2 lectins (SNA, RCA) plus anti-IgG probes simultaneously on one μMAP chip. The results of this are shown in Fig. 5E and F. Each datapoint represents properties of antibodies targeting one specific antigen, with the X value representing the titer of antigen-specific IgG and the Y value representing the level of glycans as measured via lectin binding for that antigen-specific Ab. While protein L is a positive control that binds all Abs, the other three antigens here were chosen because healthy donors are expected to have antibodies against them due to childhood vaccination (tetanus) or common prior infection (CMV, SARS-CoV-2 or other endemic human coronaviruses). For the sialic acid-modified samples, the MFI of IgG remains similar between the two groups while the MFI of SNA decreased significantly for antibodies after sialic acid removal (Fig. 5E). As the slope of the connecting line represents a change in SNA quantity over change in IgG titer, the close-to-vertical lines in Fig. 6E indicated the difference in SNA–IgG ratio matched the property of the two samples due to sialic acid cleavage and was accurately captured by the μMAP chip, validating its ability to measure the level of Fc N-glycosylation. Tetanus-specific IgG was the only exception, where a small decrease in IgG MFI was also observed after sialic acid removal. We suspect that the antigen-binding Fab region in this case had been affected by the sialic acid removal process. The same validation was observed for agalactosylated samples when tested with RCA binding on the μMAP chip (Fig. 5F). This establishes the key ability of the μMAP chip to perform multiplexed antigen-specific Ab glycoprofiling from small volumes (1000 times lower than for MS) of serum samples.
We first verified if Ab Fc receptor binding could be quantified in Schisto patient serum samples by measuring the MFI of SEA-specific antibodies that had affinity with FcR2A (Fig. 6A) and FcR2B (Fig. 6B) in pooled serum samples. Clear sample dilution-dependent response curves were formed with trends matching the nature of the samples. The two infection groups had higher MFI compared to endemic healthy controls. Next, we screened 12 individual patient serum samples from the 3 groups (C, F, H) against a set of 5 S. mansoni antigens (SEA, SM25, MEG, CD63, Calumenin B), 2 control antigens and 4 probes (IgG, IgG4, FcR2A, FcR2B) on one μMAP chip (Fig. 6C). After 2 h of assay and subsequent data processing (total <3 h), we obtained the MFI readouts from ∼1000 antigen–antibody–probe combinations, i.e., coupled Fab and Fc combinations, and used these data to evaluate potential biomarkers. The full Ab dataset is included in Fig. S6–S8.† Analyzing these data, we found that while SEA-specific IgG was low for endemic controls (SEA−Egg−), it was high in both current (SEA+Egg+) and former infected individuals (SEA+Egg−). Thus SEA-specific IgG alone could not differentiate between current and former infections (Fig. 6D, left), consistent with prior studies. By contrast, SEA-specific IgG4 successfully differentiated current from former infection (Fig. 6D, middle). This suggested that the amount of SEA-specific IgG4, an IgG subclass and an antibody Fc feature, could be a promising biomarker that differentiates different stages of schistosome infection. The MFI of the SEA antibody-IgG4 combination obtained from the μMAP chip yielded a strong correlation of R = 0.9930 with that obtained from the bead-based assay readouts (Fig. 6E), further validating the reliability of the μMAP chip when applied on individual patient serum samples. Antibodies specific to other antigens yield less difference when compared between these groups (Fig. S6–S8†). Although the other suspected Fc features tested here (Ab affinity against FcR2A/2B) did not differentiate current active from former infections in these samples (Fig. 6D, right), the MFI from the μMAP chip again yielded a strong correlation with results from bead-based assays (Fig. 6F), indicating that the μMAP chip also had the ability to measure other Ab Fc features in individual serum samples.
Overall, the μMAP chip has several distinct advantages compared to existing solutions for Ab Fc biomarker discovery. By using a highly multiplexed microarray and microfluidic channels, it requires far less sample (100–1000 times lower volume), labor and cost compared to conventional MS and ELISA (Table S1†). This sample volume reduction represents a critical enabling advantage in Ab Fc biomarker discovery for many disease contexts, where potentially large numbers of antigen specificities may have to be screened to find the right set of Ab Fab and Fc features that can act as the most accurate biomarker with high sensitivity and specificity in distinguishing specific infection or disease states.
Compared to other approaches that combine microfluidics and microarrays for Ab detection,19,29 this work is, to the best of our knowledge, the first to target not only Ab titer but also Ab Fc features including N-glycosylation and Fc receptor binding. The μMAP chip does have some unique trade-offs as well when compared to traditional microfluidics. These are the result of conscious unique design choices made here to make it more appropriate for its target use settings. The assay time (<3 h) and level of manual operations of the μMAP chip are still closer to those of a lab-based ELISA when compared to automated microfluidic approaches.20,22 While some simple manual operations are still required, the μMAP platform focuses on simplifying and reducing the cost and expertise requirement of device preparation and fabrication: instead of requiring automated valves/pumps/magnetic actuators and controlling electronics, the device only uses thin laser-cut PDMS sheets and a glass slide. The PDMS sheets required for each device are commercially available, can be patterned with cleanroom-free procedures in 2 min, and cost less than $1.5 each, whereas PDMS components in traditional automated microfluidics require soft lithography, molding and other modifications, taking significant expertise and days to fabricate. In using this platform, though there are additional steps required after sample addition, those steps such as slide washing and thin-film adhesion are commonly within the existing expertise of clinical research laboratories that routinely perform ELISAs. Thus, the μMAP platform may be especially appropriate for use in clinical or public health laboratories in resource-limited regions. The proposed μMAP workflow starts with microarray slides and PDMS sheets which can be batch produced, remain stable under proper storage, then sent to research labs in resource-limited regions that can use local serum samples to perform the assay for biomarker discovery. In such regions where infectious diseases are prevalent, but shipping samples internationally is restricted, it may be reasonable to sacrifice some level of automation in exchange for significantly reducing the cost and the required additional hardware, such as syringe or peristaltic pumps etc. and the learning curves associated with device use and maintenance.
We also note that while a microarray scanner is used here, which is not common equipment in resource-limited regions, this is not a critical requirement for the operation of this chip. Various prior works have shown portable or easy-to-fabricate versions of smartphone-based fluorescence readers,21,30–32 which can be adapted for use with this device and even enable fully automated readout by incorporating inexpensive automation approaches also available in the open hardware literature. Indeed, integration with such readout and automation approaches would form part of the future work for further development of this platform to enable deployment and use in resource-poor settings.
An additional comparison can be made here with recent pathogen detection-based assays where with the advance of microfluidic bioassays, especially by integrating PCR, pathogen detection assays have been sensitive enough to detect disease presence,33,34 even in multiplexed35 or lateral flow formats,36,37 which greatly reduces their cost. μMAP is complementary to pathogen-based biomarker detection technology (e.g. antigen detection tests such as CAA for schistosomiasis) as antibody Fc modifications still offer a unique disease-state-specific perspective in complement to direct pathogen detection. Though their use for detecting acute disease onset still needs further work, antibody Fc properties offer long-term monitoring and disease state differentiation,8,9 which often cannot be done based on the abundance of pathogens in the body alone38 and are where antigen tests often show less ideal performance.
We demonstrated the performance of the μMAP platform verifying its specificity, high dynamic range, low LOD and high correlation in comparison with existing methods. Finally, we applied it to clinical patient serum samples to discover biomarkers that differentiate active or current schistosome infection from former or non-patent infections and endemic healthy controls. Beyond this application, the platform is compatible with measuring the same type of interaction measurable by other binding assays without the use of additional sample preparation. Several limitations are related to the principle of the binding-based assays, especially those conducted on 2D surfaces such as the glass slide surface here, including the limited binding capacity per antigen and potential interactions and variants present in serum, such as soluble antigens. Future work includes performing biomarker discoveries for other endemic diseases in the field or in other laboratories, increasing the number of samples that can be tested per device by modifying channel width or substrate size, incorporating pre-printed probes39 and further improving usability by incorporating feedback from user studies. Additionally, harnessing the ability of the μMAP platform to generate high-dimensional datasets that can be coupled with modern artificial intelligence/machine learning approaches represents an exciting future prospect as well.
Footnote |
† Electronic supplementary information (ESI) available. See DOI: https://doi.org/10.1039/d5lc00042d |
This journal is © The Royal Society of Chemistry 2025 |