Cell surface glycans
are essential for establishing cell communication,
adhesion, and migration. However, it remains challenging to obtain
cell surface-specific information about glycoconjugate structures.
Acquiring this information is essential for unraveling the functional
role of glycans and for exploiting them as clinical targets. To specifically
analyze the N-glycoprotein forms expressed at the
cell surface, we developed a C18 liquid chromatography (LC)-mass spectrometry
(MS)-based glycoproteomics method in combination with highly specific
cell surface protein labeling and enrichment using a biotin label.
The surface-specificity of the method was validated by MS-based proteomics
of subcellular component marker proteins. Using the human keratinocytes
N/TERT-1 as a model system, we identified and quantified the glycosylation
of hundreds of cell surface N-glycosylation sites.
This approach allowed us to study the glycoforms present at the functional
relevant cell surface, omitting immaturely glycosylated proteins present
in the secretory pathway. Interestingly, the different stages of N-glycan processing at individual sites displayed at the
cell surface were found to correlate with their accessibility for
ER-residing processing enzymes, as investigated through molecular
dynamics simulations. Using the new approach, we compared N-glycosylation sites of proteins expressed on the cell
surface to their counterparts in a total cell lysate, showing profound
differences in glycosylation between the subcellular components and
indicating the relevance of the method for future studies in understanding
contextual glycan functions.