Experimental Analysis of Tear Fluid and their Processing for the Diagnosis of Multiple Sclerosis

Tomeckova V1
*, Tkacikova S1
, Talian I1
, Fabriciova G2
, Hovan A2
, Kondrakhova D3
, Zakutanska K4
, Skirkova M5
, Komanicky
V3
and Tomasovicova N4
1
Department of Medical and Clinical Biochemistry, Faculty of Medicine, Pavol Jozef Šafárik University in Košice, Slovakia
2
Institute of Physics, Department of Biophysics, Faculty of Science, Pavol Jozef Šafárik University in Košice, Slovakia
3
Institute of Physics, Faculty of Science, Pavol Jozef Šafárik University in Košice, Slovakia
4
Institute of Experimental Physics, Department of Magnetism, Slovak Academy of Sciences, Slovakia
5
Department of Opthalmology, Faculty of Medicine, Pavol Jozef Šafárik University in Košice, Košice
*
Corresponding author:
Vladimíra Tomečková,
Department of Medical and Clinical Biochemis-
try, Faculty of Medicine, Pavol Jozef Šafárik
University in Košice, Trieda SNP 1,
040 11 Košice, Slovakia
Received: 05 May 2023
Accepted: 05 June 2023
Published: 15 June 2023
J Short Name: COS
Copyright:
©2023 Tomeckova V, This is an open access article dis-
tributed under the terms of the Creative Commons Attri-
bution License, which permits unrestricted use, distribu-
tion, and build upon your work non-commercially.
Citation:
Tomeckova V. Experimental Analysis of Tear Fluid and
their Processing for the Diagnosis of Multiple Sclerosis.
Clin Surg. 2023; 9(6): 14
Experimental Analysis of Tear Fluid and their Processing for the Diagnosis of
Multiple Sclerosis
Clinics of Surgery
Research Article ISSN: 2638-1451 Volume 9
clinicsofsurgery.com 1
1. Abstract
A pilot analysis of the tear fluid of patients with multiple sclero-
sis (MS) collected by glass microcapillary was performed using
various experimental methods: liquid chromatography-mass spec-
trometry, Raman spectroscopy, infrared spectroscopy, and atomic
force microscopy. Infrared spectroscopy found no significant dif-
ference in both MS patients and control spectra of tear fluid; all
three significant peaks were located at around the same position.
Raman analysis showed the differences between the spectrum of
tear fluid of the MS patients and the spectrum of healthy subjects,
which indicate a decrease in tryptophan and phenylalanine content
and changes in the relative contributions of secondary structures
of polypeptide chains of tear proteins. Atomic force microscopy
exhibited a surface fern-shaped dendrite morphology of the tear
fluid of patients with MS with lower roughness on both oriented
silicon (100) and glass substrates compared to the tear fluid of con-
trol subjects. Results of liquid chromatography-mass spectrometry
showed downregulation of glycosphingolipid metabolism, sphin-
golipid metabolism, and lipid metabolism. The proteomic analy-
sis identified the up-regulated proteins in the tear fluid of patients
with MS-like cystatine, phospholipid transfer protein, transcobal-
amin-1, immunoglobulin lambda variable 1-47, lactoperoxidase,
ferroptosis suppressor protein 1; the down-regulated proteins
like haptoglobin, prosaposin, cytoskeletal keratin type I pre-mR-
NA-processing factor 17, neutrophil gelatinase-associated lipoca-
lin, and phospholipase A2.
This study showed that the tear proteome in patients with MS is
modified and can reflect inflammation. Tear fluid is not a common-
ly used biological material in clinico-biochemical laboratories.
Experimental proteomics has the potential to become a promising
contemporary tool for personalized medicine, and it might be ap-
plied in clinical practice by providing a detailed analysis of the tear
fluid proteomic profile of patients with MS.
2. Introduction
Multiple sclerosis (MS) is an autoimmune-mediated, neurodegen-
erative disorder of the central nervous system (CNS) characterized
by inflammatory demyelination with axonal transection. MS is the
most common cause of non-traumatic neurological disability in
young adults [1]. The progressive chronic inflammation leads to
the formation of multiple foci of demyelinated lesions in the white
and gray matter and finally to disability [2]. The diagnosis of MS
and evidence of dissemination in time and space are mostly based
on clinical evaluation, neuroimaging by magnetic resonance imag-
ing, and cerebrospinal fluid analysis, but no definitive diagnostic
Keywords:
Tear fluid; Multiple sclerosis; Raman spectroscopy;
Infrared spectroscopy; Proteomics; Atomic force
microscopy

Volume 9 Issue 6 -2023 Research Article
test exists [3, 4].
MS symptoms vary according to the location of lesions occurring
within the CNS [5, 6]. The most common clinical presentations
are unilateral optic neuritis, brainstem, and spinal cord syndromes
[7]. Ocular symptoms may occur at any stage of the disease. Their
course can be clinically latent or very intensive [8, 9].
Tears lubricate the ocular surface, carrying secreted molecules
from corneal epithelial cells [10]. Tears represent the whole phys-
iological status of the body [11, 12]. Quantitative determination of
tear proteins by examining all three tear fluid layers—lipid, aque-
ous, and mucous—is of increasing interest in ophthalmology [13].
In tear research and diagnostics, tear collection is a critical step.
Precorneal tears, as a biological fluid, are easily accessible with
non- or very low-invasive methods at a relatively low cost. The
complexity of tear fluid composition is a challenge for researchers
[14]. The total protein concentration of human tears ranges from 6
to 11 mg/mL, with lysozyme being the most abundant tear protein
with a concentration of approximately 1 mg/mL [15]. The main
components of human tears are proteins, as well as tear lipids, me-
tabolites, electrolytes, and vitamins [16].
The identification of protein biomarkers and molecular mecha-
nisms of MS may be elucidated by proteomics as a promising tool
for revealing molecular pathways and quantifying differentially
expressed proteins [17, 18]. Overall, proteomics, metabolomics,
and bioinformatics approaches can develop different diagnostic as-
pects of complex disorders such as MS, from biomarker discovery
to personalized medicine [4].
Tears as a non-invasive strategic material for the search for new
protein biomarkers of the nervous system seem to be an innovative
tool for the early non-invasive diagnosis of nervous system diseas-
es [19]. HPLC proteomic experimental analyses and infrared (IR)
and Raman spectral data analyses of tear fluid are shown in this
paper. This pilot study, analysed the challenges of using different
proteomic experimental analytical approaches in complex tear flu-
id of patients with MS compared with control subjects.
3. Materials and Methods
3.1. Patients and Biological Material
In this pilot study, basal tear fluid from the lower eyelid of random
patients with MS (n = 20) and healthy subjects (CTRL, n = 10)
was collected by glass microcapillary (Drummond, Broomall, PA,
USA) at the Department of Ophthalmology, University Hospital
Louis Pasteur in Košice. Before measurement, the obtained sam-
ples of tear fluid were kept at -80 °C. Table 1 provides a thorough
description of patients, procedures, and therapies. Milgamma and
vitamins B and D were given to the patients as supplements, and
they received care in accordance with the Helsinki Declaration.
They signed the informed consent form after being made aware of
the study´s goals and dangers. The revised 2017 McDonald crite-
ria, which include the history, clinical manifestations, laboratory
findings (cerebrospinal fluid-CFS), and data from neuroimaging,
were used to make the diagnosis of MS. Many patients and this
study both present the “relapsing-remitting” concept of MS. Ex-
acerbations and remissions are the hallmarks of this type of MS,
which can progress into “secondary progressive” MS with grow-
ing disability in between episodes. Relapsing-remitting, primary
progressive, and secondary progressive are the three main pres-
entation patterns for MS, a chronic autoimmune disease of the cen-
tral nervous system. The disability in “primary progressive” MS
progresses right away.
The study received clearance from the Louis Pasteur Universi-
ty Hospital in Košice’s ethics committee (protocol code 2020/
EK/06042 and date of approval: June 25, 2020) for experiments
utilizing human tear fluid.
Table 1: Description of healthy subjects (CTRL) and patients with MS.
Average CTRL MS
Patients 10 20
Females/Males Oct-00 18/2
Age (years) 26.8 ± 3.02 33.3 ± 5.3
Retinal nerve fiber layer (μm) - 101.4 ± 15.8
Ganglion cell complex (μm) - 90.5 ± 11.9
Medication 0 20
No Medication 10 -
REBIF (interferon β-1a) - 10
AVONEX (interferon β-1a) - 7
TECFIDERA (dimethyl fumarate) - 1
OCREVUS (ocrelizumab) - 2
3.2. Atomic Force Microscopy
Atomic force microscopy (AFM) is a technique that allows ob-
taining high-resolution images of any surface by using a sharp
tip scanning probe. AFM is widely used for measurements of the
morphology and roughness of various biomaterials [21,22]. AFM
is an ideal tool in interdisciplinary research to detect and study
pathological conditions even in the earliest stages.
In this study, tear fluid (5 µl) of patients with MS (n = 5) and he-
althy subjects (n = 5) was analysed by AFM analysis using atomic
force microscope (ICON, Bruker, Berkley, California, USA) in
tapping mode with silicon tips (MicroMasch, Berkley, California,
USA, NSC35 series) and the radius of curvature of 10 nm on two
different substrates: microscopic glass (with a size of 3 x 8 cm)
and oriented silicon (100) substrate (with a size of 1 x 1 cm). Tear
fluid (5 µl) was dripped on the substrate without smearing, and it
was dried at room temperature without fixative [23]. Data were
processed using ScanAsyst™ software.
3.3. Infrared Spectroscopy
Infrared spectra were acquired by FTIR spectroscope Vertex 80-v

(Bruker). Experimental (n = 6) and control samples (n = 6) were
prepared by the following procedure. Tear fluid (10 µl) obtained
by glass capillary method was deposited on a ZnSe base and dried
in a refrigerator. After drying a drop of the sample other drop or
tear fluid with a volume of 10 µl was deposited on top of the dry
layer to obtain the thicker layer of the sample. After drying the
second layer in a refrigerator the infrared spectra were measured in
transmission mode in a vacuum at ambient temperature.
3.4. Drop-coating deposition Raman spectroscopy
In drop-coating deposition Raman (DCDR) measurements, 1,5
μl of the analyte (CTRL, n = 7; MS, n = 8) was dropped on a
m-RIM™
plate (BioTools, USA) and left to dry at room tempera-
ture for about 40 min.
All spectra were obtained with a Raman confocal microspectrome-
ter (Renishaw inVia, Great Britain) equipped with a Leica direct
microscope, an electrically cooled CCD camera, and 1800 lines/
mm diffraction grating. Before the measurements, the system was
calibrated and monitored by using a silicon reference (520.5 cm-1
).
The laser beam was operated at the wavelength λ = 532 nm wa-
velength and 2 mW power to avoid heat-induced degradation of
the sample. The beam was focused onto the specimen using a
50x/0.50 NA objective, which was used to collect the Raman sig-
nal in so-called backscattering geometry. An acquisition time of
10 x 20 s was used for each spectrum. For every sample, different
spectra were measured at various locations in the dry sample to ac-
count for concentration gradients and inhomogeneities caused by
protein segregation during water evaporation. Raman spectra were
background-subtracted and normalised for clarity of presentation
and better comparison. The background was subtracted using the
rolling ball algorithm [20]. After the background subtraction, the
data were normalised to the phenylalanine peak maximum at 1003
cm-1
and/or to the peak area of the amide group at 1680 cm1
. Com-
parable results were obtained by normalising the spectra for both
bands. Almost identical results were obtained using both bands for
normalising the spectra. The average of the normalised spectra of
the control group was subtracted from each normalised spectrum
of the tear sample to obtain the difference spectra.
3.5. HPLC Mass Spectrometry
Tear fluid (15 µl) was diluted with 15 µl of 8 M urea in 0.05 M
ammonium bicarbonate. Reduction of disulfides to dithiols in tear
fluid proteins was performed with the addition of 5 mM final con-
centration of dithiothreitol (BioRad) and incubation for 30 min at
37°C. The alkylation by using 14 mM final concentration of iodoa-
cetamide (BioRad), for 30 min at 37 °C took place in the dark. The
tear fluid proteins were reduced and alkylated to break disulfide
bridges and ‚cap‘ the reduced cysteines. The urea concentration
was lowered to 0,8 M by adding 0,001 M CaCl2
. In the next step,
tear fluid proteins were digested using 0,5 µg trypsin (Promega)
per sample, overnight at 37 °C. The digestion with trypsin was
stopped by adding of 20% formic acid (Merck) to obtain pH ≤
3. Acetonitrile (3 µl) was added to tear fluid and centrifuged at
14000 x g, 4 °C, for 20 min. The supernatant (2 µl) was injected
into a nano HPLC system, Ultimate 3000 RSLC NCP (Thermo
Scientific, USA), coupled with AmaZon speed ETD ion trap mass
spectrometer (Bruker Daltonik, Germany) for proteome profiling.
Peptides were preconcentrated on the trap column Acclaim Pep-
Map 100 (Dionex, Thermo Scientific, USA), 100 µm x 2 cm, C18,
5 µm particles with water-acetonitrile loading solvent in ratio 2:98
v/v containing 0.1% formic acid at flow 8 µl.min-1
. The peptides
were then eluted and separated on a homemade capillary column
75 µm x 30 cm, packed with reversed phase C18, 3 µm particles
(Magic C18 AQ, Michrom Bioresources, USA). Mobile phases
consisted of 0.1% formic acid in a water-acetonitrile mixture in
the ratio 98/2 v/v (A) and 0.1% formic acid in the water-acetonitri-
le mixture in the ratio 5/95 v/v (B) operated at a constant flow rate
of 0.3 µl per minute. The samples were measured in auto MS/MS
mode with 10 precursors for 1 MS scan; only 2+ and 3+ precursors
were taken for fragmentation with an active exclusion set to 0.5
min. The ICC target was set to 400,000 for MS and MS/MS scans,
the maximum accumulation time was 0.050 s for MS and 0.1 s
for MS/MS. The isolation window was set to 2.2 Da, and the scan
range was 300–1,300 Da.
The Mascot 2.4 (Bruker, Germany) search engine against the
Swiss-Prot database was used to identify proteins. The parameters
were determined as follows: taxonomy – Homo sapiens (human),
variable modification: oxidation of methionine, fixed modification:
carbamidomethylation of cysteine; MS tolerance: 0.6 Da; MS/MS
tolerance: 0.6 Da; the false discovery rate (FDR) threshold was
set to 1%.
The pathway enrichment analysis (PEA) was performed by Reac-
tome Analysis Service (https.reactome.org) from the comparison
of 5 patients with MS versus 5 controls. Each sample was measu-
red twice, and at the end, 10 versus 10 measurements were analy-
sed.
4. Results
4.1. Infrared Spectroscopy
Infrared spectroscopy is a suitable method for exploring protein
structure. Infrared spectra of proteins have 9 characteristic peaks:
Amide I – Amide VII, Amide A, and Amide B. The most signifi-
cant and least complex peaks are Amide I (located at 1600 cm-1
–
1700 cm-1
), which corresponds to C-O stretching, Amide II (loca-
ted at 1480 cm-1
– 1575 cm-1
), which corresponds to N-H bending,
and C-N stretching; and Amide A (located at about 3300 cm-1
),
which corresponds to N-H stretching [24].
Representative infrared spectra of healthy controls and patients
with MS are shown in Figure 1. There were found no significant
differences between the spectrum of healthy control and MS. In
both spectra, all three significant peaks are present, and located at
around the same position.

The positions of Amide A, Amide I and Amide II peaks are listed
in Table 2. The average values for healthy controls (n = 6) and for
patients with MS (n = 6) differed by at most 2 cm-1, and the in-
tervals in which the peaks are located for MS overlap the intervals
for healthy controls (Figure 2). Infrared spectroscopy suggests no
changes in proteins visible by infrared spectroscopy in the pres-
ence of MS. No changes in the measured infrared spectra of pa-
tients with MS can be caused by small concentrations of proteins
affected by MS, whose signal is dominated by the signal of more
concentrated proteins.
Table 2: Positions of peaks Amide A, Amide I, and Amide II for CTRL and for patients with MS.
Amide A Amide I Amide II
Frequency (cm-1
) Frequency (cm-1
) Frequency (cm-1
)
CTRL
3299 1658 1543
3295 1653 1543
3298 1657 1542
3297 1658 1545
3296 1660 1548
3295 1661 1548
Average: 3297 1658 1545
MS
3295 1658 1547
3295 1658 1547
3300 1658 1541
3297 1656 1543
3296 1656 1541
3299 1657 1540
Average: 3297 1657 1543
Figure 1: Representative spectrum of tear fluid from healthy subjects and
patients with MS. Denoted values correspond to peaks Amide A, Amide I,
and Amide II, from left to right, respectively. Figure 2: Positions of peaks Amide A, Amide I, and Amide II for healthy
controls and for patients with MS. The size of the symbol reflects the
number of spectra with a given peak position. Frequency intervals for MS
overlap with intervals for healthy controls (see the x-axis). No quantity is
plotted on the y-axis, data points for MS were plotted under data points for
healthy controls for clarity.
4.2. Atomic Force Microscopy
The surface morphology of tear fluid in the control samples
(CTRL) obtained from healthy subjects as well as samples of tear
fluid with MS was studied on two different substrates (oriented
silicon (100) substrate and microscopic glass slide) by the AFM
method (Figures 4-5).

Figure 3: Average Raman spectra obtained from tears of patients with MS and CTRL (a). The difference between spectrum MS and average CTRL (b).
The shadowed area refers to the standard deviation of the data.
Figure 4: AFM topography of tear fluid of CTRL (left) and MS (right) studied on an oriented silicon (100) substrate.
Figure 5: AFM topography of tear fluid from CTRL (left) and MS (right) studied on a microscopic glass slide.
4.3. Drop-Coating Deposition Raman (DCDR) Spectroscopy
For Raman analysis, each tear fluid sample was dried on the hy-
drophobic surface to form the coffee-ring pattern to concentrate
the weak protein solution. The Raman signal of the hydrophobic
surface has a negligible effect on the Raman spectra of tear fluid.
Figure 3a shows the normalised Raman spectra of tears in the
range 400-1750 cm-1 for patients with MS and healthy controls.
The solid line represents the average Raman spectrum, and the
shaded area represents a standard error. The spectra of both groups
(MS and CTRL) have the same position of peaks.
The most intense bands in the spectra are primarily associated with
the vibrations of amide bonds and functional groups of aromatic
amino acids. Well-defined bands in the spectra correspond to vi-
brations of the phenylalanine ring (620, 1002, and 1616 cm-1),
tryptophan ring (757, 877, 1125, doublet 1336/1358, and 1554
cm-1), tyrosine ring (641, doublet 829/853, 1155, 1172, and 1616
cm-1), and amide group (1242, 1263, and 1666 cm-1) [25-27]. The
positions of the amide bands reflect the secondary structure of the
protein. Typical wavenumbers for α-helix and β-sheet structures
are 1655-1662 and 1264-1272 cm-1 (α) 1672-1676 and 1227-1242
cm-1 (β) for amide I and amide III modes, respectively [25]. This is
consistent with the fact that tear fluid contains proteins possessing
α-helix and/or β-sheet structures, such as lysozyme, lactoferrin,
and lipocalin. A broad peak near 1448 cm-1 originates from the
deformation motion of CH2 and CH3 groups, and a band around
935 cm-1 corresponds to a backbone N−Cα−C stretching vibration
of α-helix secondary structures [28]. In the Raman spectrum of
tears, we also observe less intense bands belonging to S−S stretch-
ing (505, 520, and 539 cm-1) (Table 3).
The average difference spectra of the MS and control tear fluid
samples are shown in Figure 3b. The minima occurring at 761,
1004, 1358, 1554, and 1615 cm-1 indicate a decrease in trypto-

phan and phenylalanine level content in the tear fluid of MS pa-
tients (Table 3).
Another minimum in the difference spectrum is observed at 509
cm-1 (Figure 3b), which is probably caused by a decrease in the
content of proteins containing disulphide bridges. In addition, the
minimum at 1650 cm-1 and the relative maximum at 1220 cm-1
in the difference spectrum (Figure 3b) indicate that in the tear fluid
of the MS patients, there is a change in the relative contribution
of secondary structures of polypeptide chains, a decrease in the
α-helix and an increase in the β-sheet structure.
Note that analysis of tear fluid samples (CTRL and MS) on two
types of substrates showed similar structures with similar types of
crystal growth and symmetry. The differences in the topography of
the samples obtained on different types of substrates are minimal.
The roughness of tear fluid on the silicon substrate was higher than
on the glass microscope slide. Tear fluid from patients with MS
showed lower roughness on both substrates compared to CTRL
tear fluid. Surface morphology shows the formation of fern-shaped
dendrites that differed in lengths of branches, thickness, and sur-
face roughness between CTRL and MS tear fluid samples.
A large surface roughness, above Ra = 300 nm was observed for
CTRL tear fluid samples studied on an oriented silicon substrate
compared to the finer structure of MS tear fluid, with a surface
roughness of about Ra = 70 nm. Crystals with an average height of
about 200 nm, dendrites with an average branch width of 10 µm
and a length of about 50-60 µm were observed on the surface of
tear fluid with MS (Figure 4). The average length of dendrites of
main branches in the CTRL tear fluid was more than 80 µm, and
the width was about 10-15 µm. The roughness of the surface was
Ra = 95 nm. The height of individual crystals reached 300 nm.
The surface roughness of CTRL tear fluid studied on a glass mi-
croscopic slide was about Ra = 59 nm, while finer MS tear fluid
showed a lower Ra = 25 nm surface roughness, a smaller average
crystal height (above 100 nm), and an average branch length of
dendrites (about 25 µm) with 3–4 nm width (Figure 5). The aver-
age 50 µm length of the main branches of CTRL tear fluid studied
on a microscopic glass slide was longer and thicker, with a width
of about 10 µm and separate crystals with a height of up to 200 nm
compared to MS tear fluid.
4.4. HPLC Mass Spectrometry - Bottom up Proteomic Anal-
ysis
These results summarize the pathway reactome analysis created
by the Reactome Analysis Service (https://reactome.org). Our
results from pathway enrichment analysis (PEA) demonstrated
that the metabolism of lipids (sphingolipid and glycosphingolipid
pathways) was downregulated (Figure 6, Table 4). All dysregulat-
ed MS tear fluid proteins (Table 5-6) were identified by weighted
gene set analysis.
Down-regulated proteins (Table 5) from PEAand up-regulated pro-
teins (Table 6) in the tear fluid of patients with MS were identified
by proteomic analysis. The top down-regulated proteins (Table 5)
were haptoglobin (HPT_HUMAN), prosaposin (SAP_HUMAN),
cytoskeletal keratin type I (K1C13_HUMAN), pre-mRNA-pro-
cessing factor 17 (PRP17_HUMAN), neutrophil gelatinase-asso-
ciated lipocalin, and phospholipase A2 (NGAL_HUMAN).
The top up-regulated proteins (Table 6) were cystatin C (CYTC_
HUMAN), phospholipid transfer protein (PLTP_HUMAN),
transcobalamin-1 (TCO1_HUMAN), immunoglobulin lambda
variable 1-47 (LV147_HUMAN), lactoperoxidase (PERL_HU-
MAN), and ferroptosis suppressor protein 1 (FSP1_HUMAN)
(Table 3) (Graphical Abstract).
Table 3: Peak position and tentative assignments of the Raman bands of human tears.
Peak position (cm-1
) Assignment Ref.
1666 Amid I: stretching C=O [25, 28, 29]
1616 Trp, Phe, Tyr: n8a
, ring stretching [25,29,30]
1554 Trp: stretching C2
=C3
, W3 mode [25,29]
1448 bending CH2
[25,28]
1358
Trp: Fermi resonance between in-plane N−C stretching and combination bands of ring out-of-plane
deformations, W7 mode
[27,29]
1336 Trp, C−Cα
−H bending, Cα
−C stretching [25,29]
1317 sh aliphatic sidechain stretching vibrations [25],
1263 sh amid III (α) [25,29]
1242 amid III (β) [25,29]
1206 Tyr: n7a
, C−CH2
, Phe [28, 29]
1172 Tyr: n9a
, CH in-plane bending [29,30]
1100/1125 stretching C−N [25],
1030 Phe [25],
1002 Phe [25],

954 Trp, Val [25],
935 stretching N−Cα
−C (α) [25,28,29]
877 Trp: benzene ring breathing and deformation N−H, W17 mode [28]
853/829
Tyr doublet: Fermi resonance between ring breathing mode and overtone of out-of-plane ring bending
mode
[25,28,29]
757 Trp: W18 mode [25,29]
641 Tyr: n6b
, ring deformation [25,30]
620 Phe: in-plane ring deformation [28]
539 S-S stretching (trans-gauche-trans) [25]
520 S-S stretching (gauche-gauche-trans) [25,29]
505 S-S stretching (gauche-gauche-gauche) [25,29]
Table 4: Top-regulated pathways including corresponding false discovery rate (FDR), average fold change (Av.FC) and the number of identified genes
(N Genes) obtained by Reactome Analysis.
Identifier Regulation FDR Av.FC N Genes
R-HSA-1660662
down 0.033 -1.662 1
Glycosphingolipid metabolism
R-HSA-428157
down 0.033 -1.662 1
Sphingolipid metabolism
R-HSA-556833
down 0.044 -1.086 3
Lipid metabolism
Table 5: List of top-down-regulated proteins with corresponding values of logarithm of fold change (logFC), p value (P.Value) and adjusted p values
(adj.P.Val).
Identifier logFC P.Value adj.P.Val
PIP_ HUMAN -0.5873613 0.000027 0.001406
SAP_HUMAN -1.6620236 0.0016957 0.0440891
PIGR_HUMAN -0.3813822 0.0045466 0.0788082
HPT_HUMAN -1.8960652 0.0067941 0.0883235
PRP17_HUMAN -1.0899125 0.0132627 0.1379316
K2C1B_HUMAN -0.6535084 0.0281095 0.1995068
K1C13_HUMAN -1.1428253 0.0276666 0.1995068
NGAL_HUMAN -0.9558929 0.0383667 0.1995068
PA2GA_HUMAN -0,8169733 0.0380019 0.1995068
CLUS_HUMAN -0.413297 0.0503125 0.2378411
Table 6: List of top-up-regulated proteins with corresponding values of logarithm of fold change (logFC), p value (P.Value) and adjusted p values
(adj.P.Val).
Identifier logFC P.Value adj.P.Val
TCO1_HUMAN 0.6126178 0.0373045 0.1995068
CYTC_HUMAN 1.0627939 0.0658102 0.2444378
PLTP_HUMAN 0.7180146 0.0641231 0.2444378
PERL_HUMAN 0.5038272 0.0763513 0.2646845
FSP1_HUMAN 0.4001445 0.2080562 0.4626503
LV147_HUMAN 0.5034786 0.307483 0.4996598
ZA2G_HUMAN 0.1295051 0.5520604 0.7176785
VP35L_HUMAN 0.2350438 0.6123376 0.761432
IGKC_HUMAN 0.0340178 0.8323604 0.9017238
B2MG_HUMAN 0.0037347 0.9874597 0.9874597

Figure 6: The simple scheme of lipid, sphingolipid, and glycolipid metabolism
Graphical Abstract
5. Discussion
Different biological samples from MS patients, including blood,
cerebrospinal fluid, and CNS tissue, have been subjected to proteo-
mic analysis. Blood, tissue, and cerebrospinal fluid are the samples
that must be collected through invasive procedures. Sweat, tears,
saliva, and urine are the non-invasive samples [19]. The CNS and
tears are linked. It is a fascinating pure body liquid, free of any pig-
ment that may interfere with spectral analysis. It was discovered
that tears contained the same proteins found in cerebrospinal fluid.
Tear fluid is a body fluid with a composition similar to cerebrospi-
nal fluid and blood. [19]. More than 1300 proteins were discovered
in the tear fluid of healthy individuals [19]. The major proteins
found in tears are lysozyme, lactoferrin, tear-specific prealbumin,
and secretory immunoglobulin A. Lysozyme has the highest con-
centration of 0.5–4.5 mg/ml [31], and it represents about 40% of
the protein content in tears [32]. The concentration of lactoferrin is
1-2 mg/ml (about 25% of total protein content) [31], and the con-
centration of tear-specific prealbumin and secretory immunoglo-
bulin A is 0.5–1.5 mg/ml (10–20%) [31] and 71 μg/ml–2.4 mg/ml
[33], respectively. Of all biomarkers of MS, only alpha-1 antichy-
motrypsin demonstrated a notable rise among promising proteins,
including proline-rich protein 4 and protein 16 homolog B [3]. Im-
munoglobulin G (IgG) was studied in tear fluid in connection with
MS [34]. The infrared signal from proteins affected by MS may be
dominated by major proteins, which result in identical spectra for
healthy subjects and patients with MS. Up-regulated immunoglo-
bulins (antibodies) were detected by HPLC MS spectroscopy. The
immunoglobulin light chain‘s variable domain‘s V region plays a
role in antigen recognition [35]. When an individual antigen binds
to the membrane-bound immunoglobulins during the recognition
phase of humoral immunity, these receptors cause the B lympho-
cytes to develop and differentiate into immunoglobulin-secre-
ting plasma cells [36]. The effector phase of humoral immunity

is mediated by secreted immunoglobulins, which remove bound
antigens. The V-(D)-J rearrangement assembles the variable do-
mains, which increases the possibility of somatic hypermutations,
allowing selective affinity for a specific antigen [37]. Pre-mR-
NA-processing factor 17 is required for pre-mRNA splicing. Di-
fferences in aberrant alternative pre-mRNA splicing are related to
the genetic risk variations for MS [38, 39].
Oligoclonal IgG bands are a characteristic sign of inflammation in
MS patients‘ cerebrospinal fluid and tear fluid. They can be used
as a diagnostic tool for individuals who may be experiencing their
first suspected demyelinating episode [34].
Infrared spectroscopy is not a suitable method for monitoring
changes in protein structure in patients with MS in contrast to
other diseases such as diabetes mellitus [23], eye diseases [40],
or depressive disorders [41], as we showed previously. Other ex-
perimental techniques, such as Raman spectroscopy, atomic force
microscopy, and especially liquid chromatography-mass spectro-
metry, are more suitable for MS.
Raman scattering is extremely responsive to changes in the secon-
dary structure of proteins and variations in the amount of amino
acid residues and their microenvironment, particularly those with
aromatic functional groups [25]. As a result, our Raman findings
point to a problem with tryptophan metabolism. This may affect
how neurotransmitters are regulated, leading to serious neurologi-
cal dysfunction [42].
Using NMR metabolomic analysis, two different metabolic pro-
files were distinguished in MS patients compared to CTRL [43].
The main metabolic changes were associated with tryptophan me-
tabolism and energy metabolism. Tryptophan levels in the serum
of MS patients were shown to be declining. Additionally, trypto-
phan levels in the cerebral fluid were shown to be lower in people
with secondary progressive MS [44].
It has been shown that dysregulation of haptoglobin (Hpt) in ce-
rebrospinalfluidcanreflectneurologicaldiseases[5].Itwassugges-
ted that MS research be conducted on the tears collected from MS
patients using glass microcapillaries to avoid cerebrospinal fluid
analysis, which requires an invasive collection [3].
Our proteomic research found that the Hpt proteins were upregu-
lated in the tear fluid of MS patients. Hpt modulates the acute pha-
se response. Hpt functions as an antioxidant and has antibacterial
properties. Under stressful circumstances, hemolysis of erythro-
cytes causes a buildup of hemoglobin (Hb) in the kidney, which
is then released in the urine. For hepatic recycling of heme iron
and avoiding kidney injury, Hpt catches and mixes with free plas-
ma Hb. Through an endocytic lysosomal breakdown route, Hb/
Hpt complexes are quickly eliminated by the macrophage CD163
scavenger receptor expressed on the surface of liver Kupfer cells.
In MS, high levels of inflammation are characterized by a rise in
IL-6, which in turn affects how Hpt is expressed. This illness also
has a connection to inflammation, and it progresses with muscle
breakdown, which has a connection to hemolysis. Due to the free
(Hb) pro-oxidative effect, hemolysis accelerates muscle destruc-
tion. A plasmatic Hpt rise, on the other hand, encourages its union
with free Hb (Hpt-Hb). Pro-oxidative action appears in tear fluid
due to the declining Hpt levels. A potential indicator of muscle
recovery is the involvement of Hpt, whose expression is dependent
on the synthesis of IL-6, in the pathogenesis of MS. In patients
with MS who are obese or have skeletal muscle degeneration, the
blood levels of Hpt are elevated. Due to the increased fragility of
erythrocytes in MS patients, Hpt serves as the first line of defense
for myelin against elevated Hb levels that are released. MS affects
the basic myelin proteins and changes the blood-brain barrier. [45].
A risk factor for MS could be elevated cystatin C levels, which
were discovered to be an independent predictor of cognitive im-
pairment. It is a possible sign of the diagnosis of MS in the ce-
rebrospinal fluid and tear fluid [46]. Amyloid-beta binding and
cysteine proteinases are both inhibited by statin C. In many inflam-
matory illnesses, excessive neutrophil degranulation is a common
characteristic. Since they are the most prevalent circulating and
first-responding innate myeloid cells, neutrophils have received
too little attention in the setting of multiple sclerosis (MS). Neutro-
phils are responsible for the release of inflammatory mediators and
enzymes like interleukin-1, myeloperoxidase, and different protei-
nases, the phagocytosis of myelin (as debris), the release of neutro-
phil extracellular traps, the production of reactive oxygen species,
the breakdown of the blood-brain barrier, and the production and
presentation of autoantigens. Numerous neuroinflammatory brain
disorders, including neurodegeneration, share the common mecha-
nism of neutrophil-driven inflammation [47, 48].
Innate immune reactions depend on active leukocytes releasing
myeloperoxidase. Myeloperoxidase generates hypochlorous acid
(HOCl) and other strong oxidants, which destroy bacteria and
other invasive pathogens. Myeloperoxidase promotes chronic in-
flammatory diseases [49]. Myeloperoxidase is a heme-containing
oxidoreductase that contributes to immune defense. On inflamed
mucous surfaces, recruited neutrophils and eosinophils, respecti-
vely, release heme peroxidases [50]. Lactoperoxidase gene dele-
tion results in tumors and multisystem inflammation in mice [51].
Adaptive and innate immune responses, as well as cell death of
oligodendrocytes and neurons and tissue damage due to oxidative
stress, were seen at different phases of MS [52]. The release of
iron from the myelin sheath during demyelination, mitochondrial
dysfunction along with subsequent energy failure, impaired oxi-
dative phosphorylation, inflammation, and the production of free
radicals by activated immune cells are examples of impaired redox
signaling [53].
Lipid peroxidation caused by excess of ROS and iron and a defi-
ciency of antioxidant glutathione (GSH) and glutathione peroxi-
dase (GPX) levels leads to ferroptosis. Dysregulated ferroptosis

contributes to neurodegeneration, tissue damage, inflammation,
and infection. ROS, iron, and lipids induce ferroptosis. During
ferroptosis, the cell membrane did not burst and form blisters.
In addition to the decreased or missing mitochondrial crests, the
outer mitochondrial membrane rips. Upregulation of ferroptosis
suppressor protein 1 inhibits ferroptosis. [6]. The mechanisms cau-
sing autoimmune disorders involve the cell death modes of ferrop-
tosis and pyroptosis [54].
An iron-trafficking protein known as neutrophil gelatinase-asso-
ciated lipocalin binds to iron, provides iron to the cell, or remo-
ves iron from the cell in innate immunity, ferroptosis, and other
processes. Iron-loaded form raises intracellular iron concentration
without causing apoptosis. Iron-free form decreases intracellular
iron levels and induces the production of the proapoptotic protein
BCL2L11/BIM and apoptosis because of interleukin-3 (IL3) de-
ficiency. Since neutrophil gelatinase-associated lipocalin causes
neutrophil infiltration, migration, and activation and can increase
T-helper 17 response, it influences neutrophil function. Investi-
gations have shown that neutrophil gelatinase-associated lipoca-
lin expression and secretion can be induced by IL-17 signaling
pathways alone or combined with tumor necrosis factor (TNF)-α
[55].
Neutrophil gelatinase-associated lipocalin is a protein that can
bind tiny hydrophobic compounds. It is a diagnostic indicator of
intrinsic organ injury, inflammation, and damaged cell necrosis
[56]. Neutrophil gelatinase-associated lipocalin affects both neu-
roinflammation and neuroprotection. In response to inflammatory
conditions, astrocytes in the brain produce and exude the majo-
rity of neutrophil gelatinase-associated lipocalin. Sequestered
neutrophil gelatinase-associated lipocalin causes the astrocytes
and microglia to become reactive and amplify the response. In
pathological conditions, iron accumulation and a ferric/ferrous ion
imbalance are the causes of apoptosis, necrosis, autophagy, and
ferroptosis. In fact, the cortex and hippocampus of people with ne-
urodegenerative disorders, such as MS, Alzheimer‘s disease, and
others exhibit iron buildup [57].
A special class of lysosphingolipid called sphingosylphosphoryl-
choline has been researched in cardiovascular, neurological, and
inflammatory diseases. Sphingosylphosphorylcholine controls
how the keratin network architecture is structured. The keratin re-
arrangement brought on by phosphorylation accounts for the lower
mechanical resilience. The intermediate filament proteins known
as keratins control cytoarchitecture, epithelial cell structural in-
tegrity, cell development, apoptosis, and cell motility in healthy
adult tissues as well as in certain disorders like MS. Inflammation
changes cell migration and motility. A bioactive lipid called sphin-
gosylphosphorylcholine causes the cytoplasm to relax, keratin fi-
laments to collapse within the nucleus, phosphorylation, and cell
migration. JNK and ERK, two members of the mitogen-activated
protein kinase family, have recently been demonstrated to facilita-
te keratin‘s perinuclear rearrangement during inflammation [58].
In neurodegenerative diseases like MS, altered lipid metabo-
lism and phospholipase A2 deregulation are the main causes of
inflammation. The enzymes known as phospholipases A2 break
down the fatty acids in the phospholipids of the membrane. Pro-
ducts include polyunsaturated fatty acids like arachidonic acid
and lysophosphocholin. Pro-inflammatory thromboxanes and le-
ukotrienes are produced by arachidonic acid via cyclooxygenases
and lipoxygenases, promoting reactive oxygen species formation.
Myelin loss and nerve tissue deterioration have been linked to ex-
cessive ROS production. Erythrocytes typically have larger dia-
meters, altered lipid metabolism, and molecular profiles, all of
which are positively connected with the development of MS. In
MS patients, prostaglandins, leukotrienes, ceramides, and sphin-
gosine levels are elevated. Ceramide promotes the accumulation
of oxygen species in hippocampus glial cells, which results in ne-
uronal death and is involved in developing neurodegenerative di-
sorders. Phospholipase A2 activation and arachidonic acid release
are linked to TNF-mediated signaling, with the latter leading to
the activation of sphingomyelinases that hydrolyze sphingomyelin
to create ceramide. This mechanism underpins the cytokine imba-
lance, which in turn alters the metabolism of phospholipids and
sphingolipids [59]. Together with glycerophospholipids, sphingo-
lipids are essential for numerous cellular processes, such as cell
division, signaling processes, apoptosis, and engagement in pro-
or anti-proliferative pathways. Sphingolipids are involved in the
etiology of MS and are highly expressed in the central nervous
system [60].
People with MS have dysregulated lipid metabolism. Regulated
lipid metabolism is important for the remyelination process [61].
Elevated phospholipid transfer activity may be the cause of redu-
ced lipid uptake and aberrant myelin lipids seen in MS patients
[62, 63]. Human tears contain phospholipid transfer proteins.
Phospholipid transfer protein can scavenge and transport phospho-
lipids straight to the tear fluid‘s surface layer. Instead of phospho-
lipid transfer protein, tear lipocalin is where most phospholipids
in tears are bonded. The phospholipid on the ocular surface can be
bound and removed by tear lipocalin [64]. Phospholipid transfer
protein mediates the exchange of phospholipids between triglyce-
ride-rich lipoproteins as well as the transfer of phospholipids and
free cholesterol from triglyceride-rich lipoproteins (low-density li-
poproteins, or LDL, and very low-density lipoproteins, or VLDL)
into high-density lipoproteins (HDL). Phospholipid transfer pro-
tein plays a significant role in HDL remodeling by facilitating the
transfer of a variety of different lipid molecules, including diacyl-
glycerol, phosphatidic acid, sphingomyelin, phosphatidylcholi-
ne, phosphatidylinositol, phosphatidylglycerol, cerebroside, and
phosphatidylethanolamine.

Prosaposin is a lysosomal protein that controls inflammation by
activating hydrolases involved in glycosphingolipid metabolism
in the lysosome [65]. All mammalian saposins are created from a
single prosaposin precursor molecule. Saposins, often referred to
as SAPs (sphingolipid activator proteins), are small, non-enzyma-
tic, low-molecular-weight lysosomal proteins that activate hydro-
lases, which are specialized lysosomal enzymes involved in lipid
and sphingolipid breakdown. The lack of saposin B causes neuro-
logic deficits such as demyelination, periventricular white matter
abnormalities, and peripheral neuropathy [68]. Overactivation of
platelet-neutrophil pairs was seen in MS-related inflammation and
its effects on immunological responses [69]. The metabolism of
cells influences their inflammatory characteristics. Prosaposin lin-
ks mTOR signaling and the expression of macrophages. Macropha-
ges have two functions in the pathogenesis of MS. By producing
inflammatory mediators involved in developing demyelination in
MS, they can have neuroprotective and growth-promoting effects
but can also cause tissue damage [70, 71]. Numerous neurodege-
nerative illnesses‘ pathogenesis is greatly influenced by chronic
inflammation. When no longer a triggering insult exists, the acute
inflammatory response ends, preventing a chronic inflammatory
state in physiological conditions. In patients with various chronic
inflammatory disorders, including MS, a neurodegenerative condi-
tion marked by persistent inflammation, several pathways control
the resolution of inflammation and pro-inflammatory NF-kB sig-
naling [72]. Inflamed and infected tissues quickly draw neutrophils
from the bloodstream, where they quickly attract other inflamma-
tory cells by releasing pro-inflammatory chemokines and cytoki-
nes. This process is essential for innate immunity. Inflammatory
conditions can result from overrecruitment. In many acute and
chronic inflammation cases, such as encephalomyelitis-MS, plate-
lets are necessary for neutrophil recruitment [73].
The primary component of secondary granules in neutrophils du-
ring the neutrophil degranulation pathway is transcobalamin. Co-
factors in circulation are cobalamins. Vitamin B12 binds to tran-
scobalamin. Acquired hyperhomocysteinemia is most frequently
caused by vitamin B12 and folate insufficiency. Cobalamin, gene-
rally known as vitamin B12, is essential for the structural and fun-
ctional integrity of the nervous system. A lack of cobalamin causes
demyelination, axonal degeneration, and ultimately irreversible
damage from axonal death. Therefore, a B12 shortage might cause
some clinical characteristics like those of MS patients. The seve-
rity of the disability and length of the illness were not correlated
with vitamin B12 insufficiency [74].
6. Conclusions
According to this study, MS patients have altered tear proteomes.
The tear proteome may be a good indicator of MS-related disor-
ders and CNS inflammation. Tear fluid is not a biological substan-
ce that is frequently employed in clinico-biochemical laboratories.
The vast diagnostic potential of such a small volume is currently
only being explored experimentally. In this research, specific ex-
perimental and computer-solved techniques for MS patients‘ tear
fluid are described. In conclusion, it is known that a variety of
conditions can raise the probability that MS will develop and prog-
ress, but the exact cause of this illness is still mostly unknown. The
development of MS is closely associated with stress and disruption
of lipid metabolism, as is common for other inflammatory neu-
rodegenerative disorders. An autoimmune inflammatory response
directed largely against the oligodendrocytes in the CNS triggers
the onset of MS and results in demyelination and inflammation.
After a period, when the oligodendrocytes‘ potential for regene-
ration is depleted, the inflammatory processes affect the neurons
themselves, causing neurodegeneration and lasting damage to the
CNS [75]. By offering a thorough investigation of the proteome
profile of MS patients, experimental proteomics has the potential
to might be used in clinical practice for the diagnosis of MS. Fi-
nally, clinical proteomic analysis techniques may develop into a
modern tool for personalized therapy.
7. Contributions
Conceptualization, V.T., M.S.; methodology, I.T., S.T., G.F., K.Z.,
N.T., D.K., V.K., A.H.; software, I.T., S.T., G.F., A.H., K.Z., N.T.,
D.K., V.K.; validation, I.T., S.T., G.F., K.Z., N.T., D.K., V.K.; for-
mal analysis, I.T., S.T., G.F., A.H., K.Z., N.T., D.K., V.K; inves-
tigation, M.S., I.T., S.T., G.F., K.Z., N.T., D.K., V.K.; resources,
N.T., V.K., G.F., I.T.; data curation, I.T., S.T., G.F., A.H., K.Z.,
N.T., D.K., V.K., V.T.; writing—original draft preparation, V.T.;
writing—review and editing, V.T., I.T., S.T., G.F., K.Z., N.T.,
D.K., V.K; visualization, V.T.; supervision, V.T., V.K., I.T., N.T.;
project administration, V.T.; funding acquisition, V.K., V.T., N.T.
All authors have read and agreed to the published version of the
manuscript.
8. Funding
This research was funded by the grant of the Slovak Research and
Development Agency under the contract APVV-20-0324 and by
the grant of the Research Agency of the Ministry of Education,
Science, Research and Sport of the Slovak Republic under Grant:
Integrative strategy in the development of personalized medicine
of selected cancers and its impact on quality of life, ITMS2014+:
313011V446.
9. Institutional Review Board Statement
The study was conducted in accordance with the Declaration of
Helsinki and approved by the ethical committee of Louis Pasteur
University Hospital in Košice, (protocol code 2020/EK/06042 and
25 June 2020 date of approval) for studies involving tear fluid of
humans.
10. Informed Consent Statement
Informed consent was obtained from all subjects involved in the
study.

11. Data Availability Statement
Not applicable.
12. Acknowledgments
We would like to thank you Monika Moravská and Marek Horňák
from Department of Opthalmology, Pavol Jozef Šafárik Universi-
ty in Košice Faculty of Medicine that they approved research of
patients with MS and healthy subjects who gifted us for collection
and research their tear fluid voluntary.
13. Conflicts of Interest
The authors declare no conflict of interest. The funders had no role
in the design of the study; in the collection, analyses, or interpre-
tation of data; in the writing of the manuscript; or in the decision
to publish the results.
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